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Integrated Management of Arthropod Pests <strong>and</strong> Insect Borne Diseases
Integrated Management of Plant Pests <strong>and</strong> Diseases<br />
Published:<br />
Volume 1<br />
General Concepts in Integrated Pest <strong>and</strong> Disease Management<br />
edited <strong>by</strong> A. <strong>Ciancio</strong> <strong>and</strong> K.G. Mukerji<br />
ISBN 978-1-4020-6060-1<br />
Volume 2<br />
Integrated Management <strong>and</strong> Biocontrol of Vegetable <strong>and</strong> Grain<br />
Crops Nematodes<br />
edited <strong>by</strong> A. <strong>Ciancio</strong> <strong>and</strong> K.G. Mukerji<br />
ISBN 978-1-4020-6062-5<br />
Volume 3<br />
Integrated Management of Diseases Caused <strong>by</strong> Fungi, Phytoplasma<br />
<strong>and</strong> Bacteria<br />
edited <strong>by</strong> A. <strong>Ciancio</strong> <strong>and</strong> K.G. Mukerji<br />
ISBN 978-1-4020-8570-3<br />
Volume 4<br />
Integrated Management of Fruit Crops Nematodes<br />
edited <strong>by</strong> A. <strong>Ciancio</strong> <strong>and</strong> K.G. Mukerji<br />
ISBN 978-1-4020-9857-4
Integrated Management of<br />
Arthropod Pests <strong>and</strong> Insect<br />
Borne Diseases<br />
<strong>Edited</strong> <strong>by</strong><br />
A. <strong>Ciancio</strong><br />
C.N.R., <strong>Bari</strong>, <strong>Italy</strong><br />
<strong>and</strong><br />
K.G. Mukerji<br />
University of Delhi, India
Editors<br />
Aurelio <strong>Ciancio</strong><br />
Consiglio Nazionale delle<br />
Ricerche<br />
Istituto per la Protezione delle<br />
Piante<br />
Via G. Amendola, 122/D<br />
70126 <strong>Bari</strong><br />
<strong>Italy</strong><br />
ciancio@area.ba.cnr.it<br />
K.G.Mukerji †<br />
University of Delhi<br />
Dept. Botany<br />
New Delhi-110007<br />
India<br />
kgmukerji@rediffmail.com<br />
ISBN 978-90-481-2463-3 e-ISBN 978-90-481-8606-8<br />
DOI 10.1007/978-90-481-8606-8<br />
Springer Dordrecht Heidelberg London New York<br />
Library of Congress Control Number: 2010921597<br />
c○ Springer Science+Business Media B.V. 2010<br />
No part of this work may be reproduced, stored in a retrieval system, or transmitted in any form or <strong>by</strong><br />
any means, electronic, mechanical, photocopying, microfilming, recording or otherwise, without written<br />
permission from the Publisher, with the exception of any material supplied specifically for the purpose<br />
of being entered <strong>and</strong> executed on a computer system, for exclusive use <strong>by</strong> the purchaser of the work.<br />
Printed on acid-free paper<br />
Springer is part of Springer Science+Business Media (www.springer.com)
PREFACE<br />
This is the last volume of the IPMD series. It aims, in a multi-disciplinary approach,<br />
at reviewing <strong>and</strong> discussing recent advances <strong>and</strong> achievements in the practice of crop<br />
protection <strong>and</strong> integrated pest <strong>and</strong> disease management. This last effort deals with<br />
management of arthropods, <strong>and</strong> is <strong>org</strong>anized with a first section on biological control<br />
in citrus orchards, a second one on advanced <strong>and</strong> integrated technologies for insect<br />
pest management <strong>and</strong> a last section, dealing with mites <strong>and</strong> their biological control.<br />
A wide <strong>and</strong> exaustive literature already covers several aspects of chemical or<br />
biological control of insects <strong>and</strong> mites, but there is still a need for a more holistic<br />
vision of management, accounting for different problems <strong>and</strong> solutions, as they are<br />
applied or developed, in different regions <strong>and</strong> cropping systems, worldwide. In this<br />
series we attempted to fill this gap, providing an informative coverage for a broad<br />
range of agricultural systems <strong>and</strong> situations.<br />
As for the other volumes of the IMPD Series, also this book is <strong>org</strong>anized in<br />
chapters mainly centered on crops, with a particular emphasis given on citrus<br />
production, which <strong>by</strong> itself covers the first section. Citrus is one of the main crops in<br />
which biological control <strong>and</strong> management of pests proved successful worldwide, <strong>and</strong><br />
the experience gained in this field may indeed result helpful for IMP efforts deployed<br />
on other crops <strong>and</strong>/or cropping systems, in other cultivated areas. Chapters grouped<br />
in Section 2 review the advancements of the integration of insect management<br />
options with other crop problems in extensive cropping systems (i.e. pecan, Chapter<br />
6), the application of remote sensing technologies (Chapter 7), the status of<br />
knowledge about plant defense compounds <strong>and</strong> their potentials (Chapter 8). For IPM<br />
of invasive species, Chapter 9 provides an update experience gained on the field to<br />
manage <strong>and</strong> counteract the Red Palm Weevil (RPW) in Egypt, a serious invasive<br />
pest spreading in all the mediterranean regions. Long-term technological solutions<br />
are described in Chapter 10, which deals with the extensive management of forests<br />
<strong>and</strong> park areas through aerial treatments of bacterial spores. Finally, in Section 3, an<br />
updated review about current knowledge on IPM through microbial control agents of<br />
mites is provided (Chapter 11), followed <strong>by</strong> a final chapter concerning features of<br />
predatory mites.<br />
In conclusion of this series, our sincere acknowledgements go to all the authors<br />
that provided, through their experience <strong>and</strong> dedication, a broad range of data on the<br />
management solutions thay studied <strong>and</strong> made available in different agricultural<br />
systems of the world. Thanks to their efforts, we hope we were able to contribute to<br />
spread the basic concepts related to the application of environment friendly <strong>and</strong><br />
sustainable management practices. Our hope is that this series will result useful <strong>and</strong><br />
helpful for interested readers <strong>and</strong> students, inspiring <strong>and</strong> supporting, at the same<br />
time, new <strong>and</strong> innovative research efforts in their daily field <strong>and</strong> laboratory work.<br />
v<br />
A. <strong>Ciancio</strong><br />
K. G. Mukerji †
CONTENTS<br />
Contributors ............................................................................................................ xv<br />
SECTION 1 - IPM IN CITRUS GROVES<br />
1 Citrus Pest Management in the Northern Mediterranean Basin<br />
(Spain, <strong>Italy</strong> <strong>and</strong> Greece) ................................................................................ 3<br />
Josep Anton Jacas, Filitsa Karamaouna,<br />
Rosa Vercher <strong>and</strong> Lucia Zappalà<br />
1. Introduction .................................................................................................. . 3<br />
2. Main arthropod pests <strong>and</strong> control strategies .................................................. 6<br />
2.1. Sampling <strong>and</strong> Monitoring ....................................................................... 6<br />
2.2. Biological Control .................................................................................. 6<br />
2.3. Chemical control .................................................................................. 21<br />
References ....................................................................................................... 26<br />
2 Main Arthropod Pests of Citrus Culture <strong>and</strong> Pest Management<br />
In Greece ........................................................................................................ 29<br />
Filitsa Karamaouna, Panagiotis Mylonas, Dimitrios Papachristos,<br />
Dimitrios Kontodimas, Antonios Michaelakis<strong>and</strong> Eleftheria Kapaxidi<br />
1. Introduction ................................................................................................. 29<br />
2. Pest Status <strong>and</strong> Control Measures ............................................................... 30<br />
2.1. The Mediterranean Fruit Fly, Ceratitis capitata ................................... 31<br />
2.1.1. Monitoring .................................................................................. 32<br />
2.1.2. Mass Trapping ............................................................................ 33<br />
2.1.3. Biological Control ...................................................................... 33<br />
2.1.4. Cultural Practices........................................................................ 34<br />
2.1.5. Biotechnical Methods. ................................................................ 34<br />
2.1.6. Chemical Control........................................................................ 34<br />
2.1.7. Recommended IPM Strategies. .................................................. 36<br />
2.2. Scale Insects ......................................................................................... 36<br />
2.2.1. Sampling <strong>and</strong> Monitoring . .......................................................... 37<br />
2.2.2. Biological Control ...................................................................... 37<br />
2.2.3. Cultural Practices ....................................................................... 38<br />
2.2.4. Chemical Control........................................................................ 39<br />
2.2.5. Recommended IPM Strategies ................................................... 39<br />
2.3. Whiteflies. ............................................................................................ 40<br />
2.3.1. Sampling <strong>and</strong> Monitoring . .......................................................... 40<br />
2.3.2. Biological Control <strong>and</strong> Cultural Practices .................................. 40<br />
vii
viii<br />
CONTENTS<br />
2.3.3. Chemical Control........................................................................ 41<br />
2.3.4. Recommended IPM Strategies ................................................... 41<br />
2.4. The Citrus Leafminer, Phyllocnistis citrella. ....................................... 42<br />
2.4.1. Sampling <strong>and</strong> Monitoring . .......................................................... 43<br />
2.4.2. Biological Control. ..................................................................... 43<br />
2.4.3. Cultural Practices ....................................................................... 44<br />
2.4.4. Chemical Control........................................................................ 44<br />
2.4.5. Recommended IPM Strategies. .................................................. 45<br />
2.5. Aphids. ................................................................................................. 45<br />
2.5.1. Sampling <strong>and</strong> Monitoring . .......................................................... 46<br />
2.5.2. Biological Control ...................................................................... 46<br />
2.5.3. Chemical Control........................................................................ 47<br />
2.5.4. Recommended IPM Strategies. .................................................. 47<br />
2.6. The Citrus Flower Moth, Prays citri .................................................... 48<br />
2.6.1. Sampling <strong>and</strong> Monitoring . .......................................................... 48<br />
2.6.2. Biological Control <strong>and</strong> Cultural Practices .................................. 48<br />
2.6.3. Chemical Control........................................................................ 49<br />
2.6.4. Recommended IPM Strategies ................................................... 49<br />
2.7. Thrips ................................................................................................... 49<br />
2.8. Mite Pests. ............................................................................................ 50<br />
2.8.1. Biological Control <strong>and</strong> Cultural Practices .................................. 51<br />
2.8.2. Chemical Control........................................................................ 51<br />
2.8.3. Recommended IPM Strategies. .................................................. 53<br />
3. Arthropod IPM in Citrus Throughout the Year ........................................... 53<br />
References ....................................................................................................... 53<br />
3 Biological Control in Citrus in Spain: from Classical to Conservation<br />
Biological Control .........................................................................................<br />
Josep Anton Jacas <strong>and</strong> Alberto Urbaneja<br />
1. Introduction. ................................................................................................ 61<br />
2. The Origins: Classical Biological Control in Citrus. ................................... 64<br />
3. Augmentation Versus Inoculation ............................................................... 65<br />
4. Fortuitious Biological Control ..................................................................... 66<br />
5. The Cornerstone: Conservation ................................................................... 66<br />
5.1. The First Step: Pesticide Side-Effect Testing ....................................... 67<br />
5.2. Alternative Host <strong>and</strong> Banker Plants. .................................................... 67<br />
5.3. Ground Cover Mangement Strategies .................................................. 69<br />
Conclusions ..................................................................................................... 70<br />
References ....................................................................................................... 70<br />
61
CONTENTS<br />
ix<br />
4 Citrus Integrated Pest Management in <strong>Italy</strong>. .............................................. 73<br />
Lucia Zappalà<br />
1. Introduction ................................................................................................. 73<br />
2. Main Pests <strong>and</strong> Their Control Methods ....................................................... 74<br />
2.1. Aonidiella aurantii (Maskell). .............................................................. 75<br />
2.2. Aspidiotus nerii Bouché ....................................................................... 79<br />
2.3. Phyllocnistis citrella (Stainton) ............................................................ 80<br />
2.4. Planococcus citri (Risso). .................................................................... 87<br />
2.5. Ceratitis capitata (Wiedemann). .......................................................... 89<br />
3. Secondary Pests ........................................................................................... 93<br />
References ....................................................................................................... 94<br />
5 Entomopathogenic Nematode Ecology <strong>and</strong> Biological Control<br />
in Florida Citrus Orchards ............................................................................................ 101<br />
Raquel Campos-Herrera, Robin J. Stuart, Fahiem El-Borai,<br />
Carmen Gutierrez <strong>and</strong> Larry Duncan<br />
1. Introduction. .............................................................................................. 101<br />
2. IPM of the Diaprepes-Phytophthora Complex ......................................... 104<br />
2.1. Diaprepes Economic Importance, Biology <strong>and</strong> Management ............ 104<br />
2.2. EPN Biology <strong>and</strong> Use in IPM Programs ............................................ 105<br />
2.3. Spatial Relationships Between Soils, Root Weevils <strong>and</strong><br />
Endemic EPNs ..................................................................................... 107<br />
3. From Augmenting to Conserving EPNs .................................................... 110<br />
3.1. Soil Food Webs <strong>and</strong> EPN Spatial <strong>and</strong> Temporal Patterns .................. 111<br />
3.2. Identifying Factors that Regulate EPN Abundance <strong>and</strong> Efficacy ...... 113<br />
Conclusions ................................................................................................... 123<br />
References ..................................................................................................... 123<br />
SECTION 2 - ADVANCED IPM TECHNOLOGIES<br />
6 Integration of Insect <strong>and</strong> Mite Management with Disease <strong>and</strong> Weed<br />
Control in Pecan Production . ..................................................................... 133<br />
James D. Dutcher, Lenny Wells, Timothy B. Brenneman<br />
<strong>and</strong> Michael G. Patterson<br />
1. Pests Impede the Versatility of the Pecan Tree ......................................... 133<br />
2. Pest Control Methods. ............................................................................... 136<br />
2.1. Insect <strong>and</strong> Mite Pest Management in Pecan Orchards. ...................... 137<br />
2.2. Pecan Disease Management. .............................................................. 140<br />
2.3. Weed Management in Pecan Orchards .............................................. 143<br />
3. Benefits of Crimson Clover <strong>and</strong> Legumes Use in Pecan Orchards. .......... 146<br />
3.1. Pecan Nitrogen Use <strong>and</strong> Compatibility with Crimson Clover............ 147<br />
3.2. Enhancement of Pest Management .................................................... 148<br />
3.3. Soil Building <strong>and</strong> Sustainability. . ....................................................... 149
x<br />
CONTENTS<br />
3.4. Wildlife Benefits ................................................................................ 151<br />
3.5. Establishment <strong>and</strong> Maintenance. . ....................................................... 151<br />
3.6. Costs <strong>and</strong> Savings .............................................................................. 152<br />
4. Integrated Pest Management in Pecan Orchards ....................................... 152<br />
References ..................................................................................................... 156<br />
7 Locust Habitat Monitoring <strong>and</strong> Risk Assessment Using Remote Sensing<br />
<strong>and</strong> GIS Technologies ................................................................................. 163<br />
Alex<strong>and</strong>re V. Latchininsky<strong>and</strong> Ramesh Sivanpillai<br />
1. Introduction. .............................................................................................. 163<br />
2. Remote Sensing, Geographic Information<br />
Systems (GIS), <strong>and</strong> Global Positioning Systems (GPS)............................ 165<br />
2.1. Remote Sensing ............................................................................... 165<br />
2.2. Information Extraction ..................................................................... 169<br />
2.3. Geographic Information Systems (GIS) .......................................... 169<br />
2.4. Global Positioning Systems (GPS) .................................................. 171<br />
3. Remote Sensing <strong>and</strong> Locust Pest Management ......................................... 172<br />
3.1. Desert Locust Biology <strong>and</strong> Habitat Requirements ............................. 173<br />
3.1.1. Habitat Mapping <strong>and</strong> Post-Damage Assessment. ..................... 174<br />
3.2. Migratory Locust Biology <strong>and</strong> Habitat Requirements ....................... 177<br />
3.2.1. Habitat Mapping <strong>and</strong> Post-Damage Assessment ...................... 177<br />
3.3. Australian Plague Locust ................................................................... 179<br />
3.3.1. Habitat Mapping <strong>and</strong> Post-Damage Assessment ...................... 179<br />
3.4. Other Locusts ..................................................................................... 181<br />
Conclusions ................................................................................................... 182<br />
References ..................................................................................................... 183<br />
8 Plant Defenses Against Insect Herbivory .................................................. 189<br />
Farha-Rehman, Fareed A. Khan, Shoeba B. Anis <strong>and</strong> S. M. A. Badruddin<br />
1. Introduction. .............................................................................................. 189<br />
2. Plant Defense Mechanisms ........................................................................ 190<br />
3. Insect Diversity <strong>and</strong> Crop Damage ............................................................ 192<br />
4. Herbivory .................................................................................................. 193<br />
4.1. Insect Herbivores ............................................................................... 193<br />
4.2. Plant Responses to Insect Herbivory .................................................. 194<br />
4.3. Plant Reaction to Previous Herbivores ............................................... 194<br />
4.4. Impact of Herbivory on Ecosystem .................................................... 195<br />
4.5. Herbivore Strategies ........................................................................... 196<br />
4.6. Simulation of Herbivory ..................................................................... 197<br />
5. Defense Strategies ..................................................................................... 198<br />
5.1. Plant Defense Strategies . .................................................................... 198<br />
5.2. Plant Receptor Molecules ................................................................... 199
CONTENTS<br />
xi<br />
5.3. Defense Genes in Plants ..................................................................... 199<br />
5.4. Tri-Trophic Plant Signalling .............................................................. 201<br />
Conclusions ................................................................................................... 203<br />
References ..................................................................................................... 205<br />
9 IPM of the Red Palm Weevil, Rhynchophorus ferrugineus ...................... 209<br />
Mohamed Samir Tawfik Abbas<br />
1. Introduction ............................................................................................... 209<br />
2. Habitat, Infestation <strong>and</strong> Damage ............................................................... 210<br />
2.1. Infestation Spreading.......................................................................... 210<br />
3. Biology ...................................................................................................... 211<br />
3.1. Morphological Characters .................................................................. 211<br />
3.2. Life Cycle ........................................................................................... 211<br />
3.2.1. Oviposition ............................................................................... 211<br />
3.2.2. Feeding ..................................................................................... 212<br />
3.2.3. Locomotion .............................................................................. 214<br />
4. Natural Enemies ........................................................................................ 214<br />
4.1. Parasitoids .......................................................................................... 214<br />
4.2. Predators ............................................................................................. 215<br />
4.3. Pathogens ........................................................................................... 215<br />
4.4. Nematodes .......................................................................................... 216<br />
5. Control ....................................................................................................... 216<br />
5.1. Chemicals ........................................................................................... 216<br />
5.1.1. Spraying.................................................................................... 216<br />
5.1.2. Injection .................................................................................... 217<br />
5.2. Aggregation Pheromone Traps ........................................................... 218<br />
5.2.1. Trap Design <strong>and</strong> Components .................................................. 218<br />
5.2.2. Trap Installation ....................................................................... 219<br />
5.2.3. Density of Traps ....................................................................... 219<br />
5.2.4. Utilization of Pheromone Traps ............................................... 220<br />
5.2.4.1. Traps Efficiency .......................................................... 220<br />
5.2.4.2. Estimating RPW Population Fluctuations ................... 222<br />
5.2.4.3. Estimating Reduction of RPW Populations ................. 222<br />
5.2.4.4. Estimating Sex Ratios ................................................. 223<br />
5.3. Entomopathogenic Nematodes .......................................................... 224<br />
5.3.1. Pathogenicity to RPW .............................................................. 224<br />
5.3.2. Field trials ................................................................................. 226<br />
5.3.3.1. Injection of Nematodes ............................................... 226<br />
5.3.3.2. Spraying Nematodes .................................................... 227<br />
Trunk Spraying ........................................................... 227<br />
5.4. Soil Treatments .................................................................................. 228<br />
5.5. Semi-Field Trials ................................................................................. 229<br />
References ..................................................................................................... 230
xii<br />
CONTENTS<br />
10 Control of Urticating Lepidoptera Outbreaks with<br />
Bacillus thuringiensis Aerial Treatments ................................................... 235<br />
Pio Federico Roversi, Leonardo Marianelli, Lorenzo Marziali,<br />
Michele Squarcini <strong>and</strong> Gianpaolo Barzanti<br />
1. Introduction ............................................................................................... 235<br />
2. Urticating Lepidoptera ............................................................................... 236<br />
3. Aerial Control ............................................................................................ 240<br />
References ..................................................................................................... 243<br />
SECTION 3 - MITES BIOLOGICAL CONTROL AND IPM<br />
11 IPM Potentials of Microbial Pathogens <strong>and</strong> Diseases of Mites ............... 249<br />
Leo P. S. van der Geest<br />
1. Introduction ............................................................................................... 249<br />
2. Virus Diseases ........................................................................................... 250<br />
3. Diseases Caused <strong>by</strong> Bacteria ..................................................................... 254<br />
4. Diseases Caused <strong>by</strong> Fungi ......................................................................... 260<br />
4.1. Zygomycota ....................................................................................... 261<br />
4.1.1. Course of Infection ................................................................... 263<br />
4.1.2. Natural Entomophthoraceous Infections .................................. 267<br />
4.1.3. Role of Neozygites floridana in the Field ................................. 268<br />
4.1.4. The Cassava Green Mite <strong>and</strong> Neozygites tanajoae ................... 269<br />
4.2. Deuteromycetes .................................................................................. 272<br />
4.2.1. Hirsutella infections in mites ................................................... 273<br />
4.2.2. Other Deuteromycetes Infecting Mites ..................................... 282<br />
4.3. Ascomycota ........................................................................................ 285<br />
5. Diseases Caused <strong>by</strong> Eukaryotic Microparasites ........................................ 286<br />
5.1. Apicomplexa Infections in Mites ....................................................... 290<br />
5.2. Microspora Infections in Mites .......................................................... 291<br />
6. Other Diseases ........................................................................................... 294<br />
6.1. Symptoms Ascribed to Poor Condition .............................................. 294<br />
6.2. Identification of Pathogens ................................................................. 295<br />
7. Prospects of acaropathogens for integrated pest management .................. 296<br />
References ..................................................................................................... 300<br />
12 IPM Strategies Through Specialist <strong>and</strong> Generalist<br />
Phytoseiids (Acari, Mesostigmata) ............................................................. 311<br />
Sauro Simoni <strong>and</strong> Marisa Castagnoli<br />
1. Introduction ............................................................................................... 311<br />
2. Concepts on Natural Enemies <strong>and</strong>/or Antagonists in IPM ........................ 313<br />
3. Why Phytoseiids? ...................................................................................... 314<br />
3.1. Mass Rearing ...................................................................................... 314<br />
3.2. Fitness <strong>and</strong> Adaptation Characters ..................................................... 316
CONTENTS<br />
xiii<br />
3.3. Life Style Types ................................................................................ 317<br />
3.4. Single or Multiple Antagonists Release ............................................ 320<br />
3.5. Cannibalism <strong>and</strong> Intraguild Predation ............................................... 321<br />
Conclusions ................................................................................................... 321<br />
References ..................................................................................................... 322<br />
Index ..................................................................................................................... 327
CONTRIBUTORS<br />
Mohamed S. T. Abbas<br />
Plant Protection Research Institute,<br />
Dokki, Cairo, Egypt<br />
Shoeba B. Anis<br />
Deptartment of Zoology,<br />
Aligarh Muslim University,<br />
202002 Aligarh, UP, India<br />
S. M. A. Badruddin<br />
Department of Zoology,<br />
Aligarh Muslim University,<br />
202002 Aligarh, UP, India<br />
Gianpaolo Barzanti<br />
Agricultural Research Council,<br />
Research Centre For Agrobiology<br />
<strong>and</strong> Pedology,<br />
Cascine Del Riccio,<br />
50125 Firenze, <strong>Italy</strong><br />
Timothy B. Brenneman<br />
Plant Pathology Department,<br />
University of Ge<strong>org</strong>ia,<br />
Tifton, GA, USA<br />
Raquel Campos-Herrera<br />
University of Florida, IFAS<br />
Citrus Research <strong>and</strong><br />
Education Center,<br />
FL 33850, Lake Alfred, USA<br />
Marisa Castagnoli<br />
Agricultural Research Council,<br />
Research Centre For Agrobiology<br />
<strong>and</strong> Pedology, via di Lanciola 12/A,<br />
Cascine Del Riccio,<br />
50125 Firenze, <strong>Italy</strong><br />
Larry Duncan<br />
University of Florida, IFAS<br />
Citrus Research <strong>and</strong> Education Center,<br />
Lake Alfred, FL 33850, USA<br />
James Dutcher<br />
Entomology Department,<br />
University of Ge<strong>org</strong>ia,<br />
Tifton, GA, USA<br />
Fahiem El-Borai<br />
University of Florida, IFAS<br />
Citrus Research <strong>and</strong> Education Center,<br />
Lake Alfred, FL 33850, USA;<br />
Plant Protection Department,<br />
Faculty of Agriculture,<br />
Zagazig University, Zagazig, Egypt<br />
Carmen Gutierrez<br />
Depto de Agroecología,<br />
Instituto de Ciencias Agrarias, CSIC<br />
Centro de Ciencias Medioambientales,<br />
28006 Madrid, Spain<br />
Josep Anton Jacas<br />
Universitat Jaume I (UJI),<br />
Unitat Associada d’Entomologia<br />
Agrίcola,<br />
E-12071 Castelló de la Plana, Spain<br />
Fareed A. Khan<br />
Department of Botany,<br />
Aligarh Muslim University,<br />
202002 Aligarh, UP, India<br />
Eleftheria Kapaxidi<br />
Benaki Phytopathological Institute,<br />
145 61 Kifissia, Greece<br />
Filitsa Karamaouna<br />
Benaki Phytopathological Institute,<br />
145 61 Kifissia, Greece<br />
Dimitrios Kontodimas<br />
Benaki Phytopathological Institute,<br />
145 61 Kifissia, Greece<br />
Alex<strong>and</strong>re V. Latchininski<br />
University of Wyoming,<br />
xv
xvi<br />
CONTRIBUTORS<br />
Department of Renewable Resources<br />
Laramie, WY 82071, USA<br />
Leonardo Marianelli<br />
CRA Research Centre for Agrobiology<br />
<strong>and</strong> Pedology, Cascine del Riccio,<br />
50125 Firenze, <strong>Italy</strong><br />
Lorenzo Marziali<br />
CRA Research Centre for Agrobiology<br />
<strong>and</strong> Pedology, Cascine del Riccio,<br />
50125 Firenze, <strong>Italy</strong><br />
Antonios Michaelakis<br />
Benaki Phytopathological Institute,<br />
145 61 Kifissia, Greece<br />
Panagiotis Mylonas<br />
Benaki Phytopathological Institute,<br />
8 Stefanou Delta str.,<br />
145 61 Kifissia, Greece<br />
Dimitrios Papachristos<br />
Benaki Phytopathological Institute,<br />
145 61 Kifissia, Greece<br />
Michael G. Patterson<br />
Department of Agronomy <strong>and</strong> Soils,<br />
Auburn University,<br />
Auburn, AL, USA<br />
Farha-Rehman<br />
Department of Botany<br />
Aligarh Muslim University,<br />
202002 Aligarh, UP, India<br />
Pio Federico Roversi<br />
CRA Research Centre for Agrobiology<br />
<strong>and</strong> Pedology, Cascine del Riccio,<br />
50125 Firenze, <strong>Italy</strong><br />
Sauro Simoni<br />
CRA Research Centre for Agrobiology<br />
<strong>and</strong> Pedology, via di Lanciola 12/A,<br />
Cascine del Riccio,<br />
50125 Firenze, <strong>Italy</strong><br />
Ramesh Sivanpillai<br />
Department of Botany <strong>and</strong> Wyoming<br />
Geographic Information Science Center,<br />
University of Wyoming,<br />
Laramie, WY 82071, USA<br />
Michele Squarcini<br />
CRA Research Centre for Agrobiology<br />
<strong>and</strong> Pedology, Cascine del Riccio,<br />
50125 Firenze, <strong>Italy</strong><br />
Robin J. Stuart<br />
University of Florida, IFAS<br />
Citrus Research <strong>and</strong> Education Center,<br />
Lake Alfred, FL 33850, USA<br />
Alberto Urbaneja<br />
Institut Valencià d’Investigacions<br />
Agràries (IVIA), Unitat Associada<br />
d’Entomologia Agrícola UJI-IVIA,<br />
E-46113 Montcada, Spain<br />
Leo P. S. van der Geest<br />
IBED, Section Population Biology,<br />
University of Amsterdam,<br />
1098SM Amsterdam, The Netherl<strong>and</strong>s<br />
Rosa Vercher<br />
Universidad Politécnica de Valencia<br />
Instituto Agroforestal Mediterráneo<br />
(UPV),<br />
46022 Valencia, Spain<br />
Lenny Wells<br />
Horticulture Department,<br />
University of Ge<strong>org</strong>ia,<br />
Tifton, GA, USA<br />
Lucia Zappalà<br />
Dipartimento di Scienze e Tecnologie<br />
Fitosanitarie, University of Catania,<br />
95123, Catania, <strong>Italy</strong>
OBITUARY NOTICE<br />
Prof. K. G. Mukerji<br />
Professor Krishna Gopal Mukerji passed away suddenly, aged 75. He was born on<br />
4th May 1934 at Lucknow as fourth child of Mr. Davendra Nath Mukerji <strong>and</strong> Mrs.<br />
Leela Mukerji. He received his early education in Lucknow <strong>and</strong> obtained his B.Sc.<br />
<strong>and</strong> M.Sc. degrees from Lucknow University in 1953 <strong>and</strong> 1955, respectively. In<br />
1955, he started his teaching career as Lecturer in Botany at Lucknow University,<br />
from where he also obtained his Ph.D. in Botany in 1962, with a thesis entitled<br />
“Microfungi of Usar Soil of India”. He was then appointed Lecturer in Botany at<br />
Banaras Hindu University in 1962, where he worked for 2 years. He then joined the<br />
Department of Botany at the University of Delhi as Lecturer (1964), to be later<br />
appointed Reader <strong>and</strong> Professor in 1969 <strong>and</strong> 1982, respectively. He became Head of<br />
the Department of Botany, University of Delhi during the years 1985–1988. During<br />
his scientific career he was actively engaged in research on different aspects of<br />
microbial ecology, with particular reference to soil fertility <strong>and</strong> plant productivity.<br />
His significant contributions concerned different areas of mycology, plant<br />
pathology, microbial ecology <strong>and</strong> biotechnology. In his research work he<br />
investigated, discovered <strong>and</strong> described several species <strong>and</strong> genera of fungi, including<br />
mycorrhizae from Indian soils. Professor Mukerji had keen interest in culture<br />
collections <strong>and</strong> received advanced training in fungal taxonomy at the<br />
Commonwealth Mycological Institute (CMI) in Kew, Engl<strong>and</strong> (1968), where he was<br />
also offered a permanent position as mycologist, in 1968. He also worked at the<br />
Institute of Seed Pathology at Copenhagen, Denmark (1974), at the Institute of<br />
Meeresforschung, Bremerhaven, Germany (1973) <strong>and</strong> at the Centraalbureau voor<br />
Schimmelcultures, Baarn, The Netherl<strong>and</strong>s (1974).<br />
As visiting professor or scientist, professor Mukerji visited various Institutes,<br />
Culture Collections <strong>and</strong> Laboratories throught America, Asia, Australia <strong>and</strong> Europe.<br />
His career lasted 40 years <strong>and</strong> included taxonomy <strong>and</strong> ecology of fungi from soil,<br />
photosphere <strong>and</strong> roots, as well as mycorrhizae, plant surface, <strong>org</strong>anic matter <strong>and</strong><br />
seeds. More than 200 students received their Ph.D. <strong>and</strong> M.Ph. degrees from the<br />
Delhi University, studying various aspects of mycology, plant pathology, microbial<br />
xvii
xviii<br />
O<br />
BITUARY<br />
N<br />
OTICE<br />
ecology <strong>and</strong> microbial biotechnology under his supervision. Professor Mukerji was a<br />
widely traveled botanist <strong>and</strong> attended several national <strong>and</strong> international conferences<br />
<strong>and</strong> symposia, presenting key notes <strong>and</strong> invited papers. He was a member of<br />
numerous societies <strong>and</strong> associations, also as Treasurer (Mycological Society of<br />
India, 1973–1976), Vice-President (Mycological Society of India, 1980–1981 <strong>and</strong><br />
Association of Tropical Microbial Ecology, 1980–1984), President (Society for<br />
Advancement of Botany, 1987, <strong>and</strong> Society for Environment scientists, 1988–1991).<br />
He was member of several editorial boards, inlcuding the Transactions of the<br />
Mycological Society of India (1979–198l), Phytologia, the Journal of the Indian<br />
Botanical Society <strong>and</strong> the Journal of Phytology Research (since 1988). He was also<br />
Editor or Advisory Committee member for several journals, including the Indian<br />
Journal of Microbial Ecology, Frontiers in Applied Microbiology, CRC Critical<br />
Reviews on Biological Control of Plant Pests, Diseases <strong>and</strong> Weeds (since 1990).<br />
Professor Mukerji was also Councillor for the International Society of Root<br />
Research <strong>and</strong> the Nitrogen Fixing Tree Association. He authored or co-authored<br />
more than 550 research papers on various aspects of mycology, plant pathology,<br />
microbial ecology <strong>and</strong> biotechnology, <strong>and</strong> co-authored, edited <strong>and</strong> co-edited more<br />
than 45 books, dealing with various aspects of microbial ecology <strong>and</strong> biotechnology.<br />
Professor Mukerji retired as Senior Professor from the University of Delhi in 2004<br />
but continued his intense editorial <strong>and</strong> publication activity until this year. As one of<br />
the most distinguished mycologist <strong>and</strong> microbial ecologist from India he is still<br />
credited for his research contributions, which are recognized all over the world. His<br />
death is a great loss for India as well as for the international scientific community.<br />
Those who had the priviledge of sharing with him some work time will remember a<br />
very gentle <strong>and</strong> kind person, <strong>and</strong> a bright, experienced <strong>and</strong> outst<strong>and</strong>ing scientist. We<br />
convene our sincere <strong>and</strong> heartfelt condolences at this most difficult of times to his<br />
beloved wife <strong>and</strong> son. He will be greatly missed.<br />
A. <strong>Ciancio</strong><br />
Zuzana Bernhart
Section 1<br />
IPM IN CITRUS GROVES
1<br />
CITRUS PEST MANAGEMENT IN THE NORTHERN<br />
MEDITERRANEAN BASIN (SPAIN, ITALY AND<br />
GREECE)<br />
JOSEP ANTON JACAS 1 , FILITSA KARAMAOUNA 2 , ROSA<br />
VERCHER 3 AND LUCIA ZAPPALÀ 4<br />
1 Universitat Jaume I(UJI),Unitat Associada d’Entomologia<br />
Agrίcola UJI-IVIA, E-12071 Castelló de la Plana, Spain<br />
2 Benaki Phytopathological Institute,<br />
14561 Kifissia, Greece<br />
3 Instituto Agroforestal Mediterráneo,<br />
Universidad Politécnica de Valencia, 46022 Valencia, Spain<br />
4 Dipartimento di Scienze e Tecnologie Fitosanitarie,<br />
University of Catania, 95123 Catania, <strong>Italy</strong><br />
Abstract. Main management options for arthropod pests of citrus <strong>and</strong> species recently introduced in the<br />
northern Mediterranean regions are reviewed. Available control strategies are discussed, including visual<br />
inspection practices, insect trapping methods <strong>and</strong> natural enemies release in augmentative or classical<br />
biological control. IPM practices <strong>and</strong> side effects of pesticides are also reviewed.<br />
1. INTRODUCTION<br />
The most widely cultivated citrus species in the Mediterranean region include<br />
orange [Citrus sinensis (L.) Osbeck], lemon [Citrus limon (L.) Burman f.], m<strong>and</strong>arin<br />
(Citrus reticulata Blanco), tangerine (Citrus deliciosa Tenore), grapefruit (Citrus<br />
paradisi Macfadyen), sour orange (syn. Chinese bitter orange, bigarade orange,<br />
Seville orange) (Citrus aurantium L.), lime [Citrus aurantifolia (Christm.) Swingle]<br />
<strong>and</strong> citron (Citrus medica L.) (Katsoyannos, 1996). Minor citrus species are pumelo<br />
(syn. shaddock) [Citrus maxima (Burm.) Merrill, syn. C. gr<strong>and</strong>is (L.) Osbeck, C.<br />
All authors contributed equally to this chapter.<br />
A. <strong>Ciancio</strong>, K.G. Mukerji (eds.), Integrated Management of Arthropod Pests<br />
<strong>and</strong> Insect Borne Diseases, Integrated Management of Plant Pests <strong>and</strong> Diseases 5,<br />
DOI 10.1007/978-90-481-8606-8_1, © Springer Science+Business Media B.V. 2010<br />
3
4<br />
J.A. JACAS ET AL.<br />
decumana L.], bergamot (Citrus bergamia Risso) <strong>and</strong> chinotto or myrtle-leaved<br />
orange (Citrus myrtifolia Raf.).<br />
The total area of citrus production in the Mediterranean region sums up to<br />
1,036,878 ha (Franco, García-Marí, Ramos, & Besrí, 2006; ISTAT, 2007; El-<br />
Otmani, Srairi, & Benhaddou, 2007; Laajimi & Ben Mimoun, 2007; MAPA, 2007;<br />
Salama Eid, Latif, & Hassan, 2007) with more than 2/3 of the entire area<br />
concentrated in Spain, <strong>Italy</strong>, Egypt <strong>and</strong> Turkey (Table 1). Integrated Pest<br />
Management is performed on a percentage of this area that varies in each country<br />
from less than 1% in France (Corsica) to 100% in Israel. In <strong>Italy</strong>, Morocco <strong>and</strong><br />
Portugal 10–20% of the total citrus production area is under IPM, while in Turkey<br />
this management strategy is applied on 30% of this area. Integrated production (IP)<br />
is only reported in Spain, <strong>Italy</strong>, Portugal <strong>and</strong> France ranging between 0.4%<br />
(Portugal) <strong>and</strong> 10% (<strong>Italy</strong>) of the total citrus area (Franco et al., 2006).<br />
Table 1. Total area of citrus production <strong>and</strong> percentage of integrated pest<br />
management (IPM) <strong>and</strong> integrated production (IP) in Mediterranean countries<br />
(modified from Franco et al., 2006. N.a. st<strong>and</strong>s for not available).<br />
Country<br />
Citrus production area<br />
(ha)<br />
IPM (%) IP (%)<br />
Spain 311,004 Most of the area 5<br />
<strong>Italy</strong> 164,938 10–20 10<br />
Egypt 151,075 n.a. n.a.<br />
Turkey 150,000 30 –<br />
Morocco 80,000 10–20 –<br />
Greece 57,526 Most of the area –<br />
Algeria 45,400 n.a. –<br />
Portugal 27,755 14 0.4<br />
Tunisia 18,600 n.a. n.a.<br />
Israel 17,300 100 –<br />
Ge<strong>org</strong>ia 11,000 n.a. –<br />
France (Corsica) 1,800
CITRUS PEST MANAGEMENT IN THE MEDITERRANEAN BASIN 5<br />
IPM/IP guidelines are defined at regional level in Greece, Portugal <strong>and</strong> Turkey,<br />
<strong>and</strong> at both regional <strong>and</strong> national level in Israel, <strong>Italy</strong> <strong>and</strong> Spain. IPM/IP certification<br />
companies are reported in <strong>Italy</strong>, Spain <strong>and</strong> Portugal (Franco et al., 2006).<br />
Guidelines for Integrated Production of Citrus have been produced <strong>by</strong> the<br />
IOBC/WPRS Commission “IP-Guidelines <strong>and</strong> Endorsement” (IOBC/WPRS, 2004),<br />
<strong>and</strong> they mainly concern st<strong>and</strong>ards for the IP <strong>org</strong>anizations in order to develop<br />
national or local guidelines. According to these st<strong>and</strong>ards <strong>and</strong> in relation to<br />
integrated plant protection, all available preventive (indirect) plant protection<br />
measures must be applied before direct control techniques are used. Priority should<br />
be given to natural, cultural, biological, genetic (GMOs are generally excluded <strong>and</strong><br />
permission may be given on a case-<strong>by</strong>-case study) <strong>and</strong> biotechnical methods of pest<br />
control <strong>and</strong> the use of agrochemicals should be minimized.<br />
The decision for the application of direct control methods must be based on<br />
economic thresholds, wherever possible, risk assessments <strong>and</strong> forecasts, including<br />
those provided <strong>by</strong> official forecasting services. A restricted list of the key pests,<br />
diseases <strong>and</strong> weeds that require regular attention must be established <strong>by</strong> the IP<br />
<strong>org</strong>anizations <strong>and</strong> their populations should be regularly monitored <strong>and</strong> recorded. In<br />
addition at least three key natural enemies in each crop must be identified in<br />
national/regional guidelines. Furthermore, the use of plant protection products toxic<br />
to these beneficial arthropods should be reduced to a minimum <strong>and</strong> always in<br />
periods of low activity of the natural enemies, or of low risk for them. Populations<br />
of key natural enemies must be preserved <strong>and</strong> incremented.<br />
With regard to pesticides, all those locally or nationally available must be<br />
classified <strong>by</strong> the IP <strong>org</strong>anizations in two lists: the “green list” including the<br />
permitted products <strong>and</strong> the “yellow list” including those pesticides permitted with<br />
restrictions. The pesticides categorization is based on several criteria (i.e. toxicity to<br />
man, toxicity to key natural enemies, toxicity to other natural <strong>org</strong>anisms, pollution<br />
of ground <strong>and</strong> surface water, ability to stimulate pests, selectivity, persistence,<br />
incomplete information, necessity of use), <strong>and</strong> it is already established for certain<br />
pesticides <strong>and</strong> pesticide groups as follows:<br />
- Not permitted: pyrethroid insecticides <strong>and</strong> acaricides, non-naturally<br />
occurring plant growth regulators (their use can only be allowed when<br />
absolutely necessary), <strong>org</strong>anochlorine insecticides <strong>and</strong> acaricides, water<br />
polluting products <strong>and</strong> very persistent herbicides;<br />
- Permitted with restrictions: dithiocarbamate fungicides (normally<br />
maximum of three applications per season <strong>and</strong> not in succession, so that<br />
predatory phytoseiid mites are not affected), fosetil-Al <strong>and</strong> phosphonate<br />
potassium (maximum of two applications per year), metalaxyl (maximum<br />
of 2 g/m 2 ), residual (soil) herbicides (except toxic, polluting or very<br />
persistent products) in the first 3 years after planting (maximum of one<br />
dose-equivalent per annum).<br />
Officially recognized dose adjustment protocols must be used where available, in<br />
order to adapt dose rates to the size <strong>and</strong> density of the target trees being sprayed.<br />
The maximum volume of application per hectare must be defined according to the
6<br />
J.A. JACAS ET AL.<br />
tree volume. A strategy of m<strong>and</strong>atory measures for minimizing the risk of resistance<br />
development of pests to pesticides (e.g. maximum number of applications per year,<br />
alternation of pesticides with different mode of action) must be set <strong>by</strong> the IP<br />
<strong>org</strong>anizations. The growers/applicators must be trained in the use <strong>and</strong> the application<br />
of pesticides.<br />
2. MAIN ARTHROPOD PESTS AND CONTROL STRATEGIES<br />
In the citrus producing countries of the Mediterranean basin more than 140 pests <strong>and</strong><br />
diseases are reported, including 108 insects, 10 mites, 1 nematode, 14 fungi, 2<br />
bacteria <strong>and</strong> 8 virus <strong>and</strong> virus like diseases (Franco et al., 2006).<br />
Among arthropods, the major pests, i.e. reported as key-pests in at least 50% of<br />
the countries, include the medfly Ceratitis capitata (Wiedemann) (100% of the<br />
countries), the California red scale Aonidiella aurantii (Maskell) (71%), the citrus<br />
leafminer Phyllocnistis citrella Stainton (71%) <strong>and</strong> the citrus mealybug Planococcus<br />
citri (Risso) (71%) (Table 2).<br />
Quarantine pests recently introduced in the western Mediterranean area include<br />
the brown citrus aphid Toxoptera citricida (Kirkaldy) (Northern Spain, from Galicia<br />
to the Basque Country, Madeira isl<strong>and</strong> <strong>and</strong> North of Portugal), the African citrus<br />
psylla Trioza erytreae (Del Guercio) (Madeira <strong>and</strong> Canary isl<strong>and</strong>s) <strong>and</strong> the citrus<br />
snow scale Unaspis citri (Comstock) (Azores, Malta <strong>and</strong> France). These species are<br />
included in the EPPO lists A1–A2 <strong>and</strong> are therefore regulated as quarantine pests in<br />
the whole EPPO region (EPPO, 2007). Special attention must be paid to T. citricida<br />
<strong>and</strong> T. erytreae as they are efficient vectors of the citrus tristeza virus (CTV) <strong>and</strong> the<br />
Huanglongbing agent (C<strong>and</strong>idatus Liberobacter), respectively.<br />
2.1. Sampling <strong>and</strong> Monitoring<br />
In IPM, pest control decisions are directly dependent upon knowing the status <strong>and</strong><br />
population trends of the most important insect pests <strong>and</strong> their natural enemies<br />
(Beardsley, AliNiazee, & Watson, 1979; Cavalloro & Prota, 1983; Katsoyannos,<br />
1996). Sampling <strong>and</strong> monitoring are the means for acquiring this important<br />
knowledge. Simplified sampling guidelines for monitoring the main citrus insect<br />
pests in the northern Mediterranean have been advised <strong>by</strong> experts defining methods<br />
of visual inspection as well as trapping using food, chromotropic <strong>and</strong> sexual<br />
attractants for monitoring purposes (Katsoyannos, 1996) (Tables 3 <strong>and</strong> 4).<br />
2.2. Biological Control<br />
Biological Control has been proved very effective in management of insect pests in<br />
citrus orchards. Among 65 cases of successful biological control <strong>and</strong> 83 cases of<br />
satisfactory control of insect pests in various crops, which have been recorded all<br />
over the world, 61.5% of the first mentioned <strong>and</strong> 21.7% of the latter concern citrus<br />
(De Bach, 1964).
CITRUS PEST MANAGEMENT IN THE MEDITERRANEAN BASIN 7<br />
Several programmes of augmentative <strong>and</strong> classical biological control <strong>by</strong> means<br />
of parasitoids <strong>and</strong> predators of the main citrus pests have been conducted in most of<br />
the northern Mediterranean citrus growing countries (Table 5). The results vary,<br />
however, several successful cases have been recorded (Viggiani, 1975; Amaro,<br />
1992; Noyes & Hayat, 1994; Katsoyannos, 1996; Tsagarakis, Kalaitzaki,<br />
Lykouressis, Michelakis, & Alex<strong>and</strong>rakis, 1999; Kalaitzaki, 2004; Siscaro, Caleca,<br />
Reina, Rizzo, & Zappalà, 2003; Siscaro, Di Franco, & Zappalà, 2008; Gomes da<br />
Silva, B<strong>org</strong>es da Silva, & Franco, 2006; Jacas, Urbaneja, & Viñuela, 2006; Malausa,<br />
Rabasse, & Kreiter, 2008; Zappalà, Siscaro, & Longo, 2008).<br />
Table 2. Arthropod pests of citrus <strong>and</strong> rating of their pest status in the northern<br />
Mediterranean regions (modified from Franco et al., 2006)*.<br />
Group Order Family Species<br />
France (F)<br />
Greece (G)<br />
<strong>Italy</strong> (I)<br />
Montenegro<br />
(M)<br />
Portugal<br />
(P)<br />
Spain (S)<br />
Turkey (T)<br />
Insects<br />
Orthoptera<br />
Acrididae<br />
Tettigonidae<br />
Thysanoptera<br />
Thripidae<br />
Hemiptera<br />
Anacridium<br />
aegyptium (L). 0 1 0 1 1 0<br />
Phaneroptera<br />
nana Fiebre 0 0 0 2 1 0<br />
Frankliniella<br />
bispinosa (M<strong>org</strong>an) 0 0 1 a 0 0<br />
Frankliniella<br />
occidentalis (Perg<strong>and</strong>e) 1 1 1 2 1 2<br />
Heliothrips<br />
haemorrhoidalis<br />
(Bouché) 1 2 b 2 1 0<br />
Pezothrips<br />
kellyanus (Bagnall) 2 2 1 b 1 2<br />
Thrips australis (Bagnall) 0 0 1 0 0<br />
Thrips flavus Schrank 1 1 2 1 0<br />
Thrips major Uzel 1 0 2 1 2<br />
Thrips tabaci Lindeman 1 1 1 2 0 2<br />
Pentatomidae Nezara viridula (L.) 1 1 0 1 0 2<br />
Miridae Closterotomus trivialis<br />
(Costa) 2 2 0 0 1,2 0<br />
Flatidae Metcalfa pruinosa (Say) 3 1 1 1 0 0<br />
Cicadellidae Empoasca<br />
decedens (Paoli) 0 1 1 0 2 c 1<br />
Triozidae Trioza<br />
Erytreae (Del Guercio) 0 0 0 3 a 2 d 0
8<br />
J.A. JACAS ET AL.<br />
Table 2 continued<br />
Group Order Family Species<br />
France (F)<br />
Greece (G)<br />
<strong>Italy</strong> (I)<br />
Montenegro<br />
(M)<br />
Portugal<br />
(P)<br />
Spain (S)<br />
Turkey (T)<br />
Aleyrodidae Aleurothrixus<br />
Floccosus (Maskell)<br />
3 2 2 1 3 2 2<br />
Bemisia<br />
afer (Priesner & Hosny) 0 1 0 0 1 0<br />
Bemisia<br />
tabaci (Gennadius) 2<br />
Dialeurodes<br />
citri (Ashmead) 3 2 e 1 3 0 1 1<br />
Dialeurodes<br />
citrifolii (M<strong>org</strong>an) 0 0 0 1 a 0 0<br />
Parabemisia<br />
myricae (Kuwana) 0 1 1 0 1 1 2<br />
Paraleyrodes<br />
bondari Peracchi 0 0 0 1 a 0 0<br />
Paraleyrodes<br />
citricolus Costa Lima 0 0 0 1 a 0 0<br />
Paraleyrodes<br />
minei Iaccarino 0 0 0 1 1 2<br />
Aphididae Aphis craccivora Kock 2 1 1 2 1 1 2<br />
Aphis fabae Scopoli 2 1 1 1 1 0<br />
Aphis gossypii Glover 3 2 2 0 3 2 1<br />
Aphis spiraecola Patch 2 2 0 3 2 1<br />
Aulacorthum<br />
solani (Kaltenbach) 2 1 1 0 1 0 0<br />
Macrosiphum<br />
euphorbiae (Thomas) 2 1 1 0 1 0 0<br />
Myzus ornatus Laing 0 0 0 1 a 0 0<br />
Myzus persicae (Sulzer) 2 1 1 1 1 1<br />
Neomyzus<br />
circunflexum (Buckton) 0 0 0 0 0 0<br />
Rhopalosiphum<br />
maidis (Fitch) 0 1 0 0<br />
Toxoptera<br />
aurantii (Boyer de)<br />
(Fonscolombe) 3 2 2 2 3 1 2<br />
Toxoptera<br />
citricida (Kirkaldy) 0 0 0 0 3 fa 2 g 0<br />
Margarodidae Icerya purchasi Maskell 3 1 1 1 2 1 1<br />
Ortheziidae<br />
Orthezia<br />
insignis Douglas 0 0 0 1 a 0 0
Table 2 continued<br />
CITRUS PEST MANAGEMENT IN THE MEDITERRANEAN BASIN 9<br />
Group Order Family Species<br />
France (F)<br />
Greece (G)<br />
<strong>Italy</strong> (I)<br />
Montenegro<br />
(M)<br />
Portugal<br />
(P)<br />
Spain (S)<br />
Turkey (T)<br />
Pseudococcidae<br />
Coccidae<br />
Diaspididae<br />
Nipaecoccus<br />
nipae (Maskell) 0 0 0 1 a 0 0<br />
Phaenacoccus<br />
madeirensis Green 0 1 0 0 0<br />
Planococcus citri (Risso) 3 3 2, 3 1 3 1, 2 3<br />
Pseudococcus<br />
calceolariae (Maskell) 0 1 0 2 1 0<br />
Pseudococcus longispinus<br />
(Targioni-Tozzetti)<br />
1 1 0 1 1 0<br />
Pseudococcus<br />
viburni (Signoret) 0 1 0 2 0 1<br />
Ceroplastes<br />
floridensis Comstock 1 0 0 1 ah 1 3<br />
Ceroplastes<br />
japonicus Green 1 1 0 0 0<br />
Ceroplastes rusci (L.)<br />
1 2 0 1 1 1<br />
Ceroplastes<br />
sinensis Del Guercio 3 1 1 1 2 1 0<br />
Coccus hesperidum L. 3 1 1 1 2 1 2<br />
Coccus pseudomagnoliarum<br />
(Kuwana) 1 1 2 0 2<br />
Coccus viridis (Green) 0 0 0 1 a 0 0<br />
Eucalymnatus<br />
tessellates (Signoret) 0 0 0 1 a 0 0<br />
Parasaissetia<br />
nigra (Nietner) 0 0 0 1 a 0 0<br />
Parthenolecanium<br />
persicae (F.) 0 1 0 1 0 0<br />
Protopulvinaria<br />
pyriformis ( Cockerell) 0 1 1 0 1,2 a 1 0<br />
Pulvinaria<br />
floccifera ( Westwood) 0 1 0 0 0<br />
Saissetia coffeae (Walker) 0 1 0 1,2 1<br />
Saissetia oleae (Olivier) 3 1 2 2 2 1 2<br />
Aonidiella<br />
aurantii (Maskell) 3 2 3 1 3 i 3 3<br />
Aspidiotus nerii Bouché 1 3 b 0 1 2 b 0<br />
Chrysomphalus aonidum (L.) 1 2 0 0 0 0<br />
Chrysomphalus<br />
dictyospermi (M<strong>org</strong>an) 3 1 1 1 2 1 2
10<br />
J.A. JACAS ET AL.<br />
Table 2 continued<br />
Group Order Family Species<br />
France (F)<br />
Greece (G)<br />
<strong>Italy</strong> (I)<br />
Montenegro<br />
(M)<br />
Portugal<br />
(P)<br />
Spain (S)<br />
Turkey (T)<br />
Lepidoptera<br />
Gracillariidae<br />
Chrysomphalus<br />
pinnulifer Maskell 0 0 0 1,2 a 0 0<br />
Hemiberlesia<br />
rapax (Comstock) 0 1 0 1 1 0<br />
Lepidosaphes<br />
gloverii (Packard) 3 0 2 0 1 1 0<br />
Lepidosaphes<br />
beckii (Newman) 3 2 1 1 3 2, 3 2<br />
Lopholeucaspis<br />
japonica (Cockerell) 0 0 0 0 0<br />
Mycetaspis<br />
personata (Comstock) 0 0 0 1 a 0 0<br />
Parlatoria<br />
perg<strong>and</strong>ei Comstock 3 1 2 0 2 2, 3 1<br />
Parlatoria<br />
ziziphi (Lucas) 0 2 2 0 0 1 0<br />
Diaspidiotus<br />
perniciosus (Comstock) 0 0 0 0 0 0<br />
Unaspis citri (Comstock) 0 0 0 0 3 h 0 0<br />
Unaspis<br />
yanonensis (Kuwana) 2 0 2 0 0 0<br />
Phyllocnistis<br />
citrella Stainton 3 2<br />
jk<br />
2 3 jk 3 j 1, 2 3 j<br />
Hyponomeutidae Prays citri (Millière) 3 2 2 b 0 3 b 3 b 1 b<br />
Tortricidae Archips rosanus (L.) 1 1 1 0 0<br />
Cacoecimorpha<br />
pronubana (Hübner) 1 1 1 2 1 2<br />
Geometridae Cleora<br />
fortunata ( Blachier )<br />
0 0 0 1 a 0 0<br />
Gymnoscelis<br />
pumilata Hübner 0 1 0 0 0<br />
Gymnoscelis<br />
rufifasciata (Haw.) 0 0 0 1 0 0<br />
Noctuidae Helicoverpa<br />
armigera (Hübner) 0 0 0 1 b 1 2<br />
Peridroma<br />
saucia (Hübner) 0 0 0 1 0 0<br />
Pyralidae Cryptoblabes<br />
gnidiella ( Millière) 1 1 0 2 1 2<br />
Ectomyelois<br />
ceratoniae (Zeller)<br />
1 1 0 2 1 2
Table 2 continued<br />
CITRUS PEST MANAGEMENT IN THE MEDITERRANEAN BASIN 11<br />
Group Order Family Species<br />
France (F)<br />
Greece (G)<br />
<strong>Italy</strong> (I)<br />
Montenegro<br />
(M)<br />
Portugal<br />
(P)<br />
Spain (S)<br />
Turkey (T)<br />
Nymphalidae Charaxes jasius L. 0 1 0 0 0<br />
Diptera<br />
Tephritidae Ceratitis<br />
capitata (Wiedemann)<br />
3 3 3 2, 3 e 3 3 3 lm<br />
Coleoptera<br />
Curculionidae<br />
Scarabaeidae<br />
Hymenoptera<br />
Formicidae<br />
Mites<br />
Acariformes<br />
Asynonychus<br />
godmani (Cratch) 0 0 0 1 0 0<br />
Lyxus algirus L. 0 0 0 2 1 0<br />
Otiorrhynchus<br />
aurifer Boheman 0 2 jk 0 0 0<br />
Otiorrhynchus<br />
cribricollis Gyllenhall 0 2 j k<br />
0 0 1 0<br />
Pantomorus<br />
cervinus (Boheman) 0 0 0 2 a 0 0<br />
Cetonia carthami<br />
0 0 0 1 0 0<br />
aurataeformis Curtis<br />
Oxythyrea funesta (Poda) 1 1 1 1 1 0<br />
Tropinota hirta (Poda) 1 1 1 1 0<br />
Tropinota squalida (Scop.) 1 1 0 1 1 0<br />
Camponotus<br />
nyl<strong>and</strong>eri Emery 0 2 n 0 0 0<br />
Crematogaster<br />
scutellaris (Olivier) 0 2 n 0 0 0<br />
Lasius niger (L.)<br />
Linepithema<br />
0 2 n 0 2 a 1 0<br />
(=Iridomyrmex)<br />
humile (Mayr)<br />
Tapinoma<br />
0 2 n 0 2 1 0<br />
nigerrimum (Nyl<strong>and</strong>er)<br />
Tapinoma<br />
0 2 0 0 0<br />
simrothi Krausse<br />
0 0 0 2 a 1 0<br />
Eriophyidae Aculops pelekassi (Keifer) 2 2 2 0 0 0<br />
Eriophyes<br />
sheldoni (Ewing) 2 2 b 1 2 b 2 b 1<br />
Phyllocoptruta<br />
oleivora (Ashmead) 1 0 0 0 0 3
12<br />
J.A. JACAS ET AL.<br />
Table 2 continued<br />
Group Order Family Species<br />
France (F)<br />
Greece (G)<br />
<strong>Italy</strong> (I)<br />
Montenegro<br />
(M)<br />
Portugal<br />
(P)<br />
Spain (S)<br />
Turkey (T)<br />
Tarsonemidae<br />
Tenuipalpidae<br />
Polyphagotarsonemus<br />
latus (Banks) 1 2 b 0 2 bk 1 2<br />
Brevipalpus<br />
californicus (Banks) 1 1 0 1 1 0<br />
Brevipalpus<br />
phoenicis (Geijskes) 1 0 0 2 1 0<br />
Tetranychidae<br />
Eutetranychus<br />
banksi (McGregor) 0 0 0 3 i o<br />
2 0<br />
Eutetranychus<br />
orientalis (Klein) 0 0 0 0 2 c 0<br />
Panonychus<br />
citri McGregor 3 2 2 3 2 2 1<br />
Tetranychus<br />
urticae (Koch)<br />
1 2 1,2 1 1 1–3 2<br />
* Ratings: 3 = key pest, requires the application of control measures most of the years because of<br />
economic damage; 2 = occasional pest, may reach economic injury level; 1= potential pest, always<br />
below economic injury level; 0 = not reported on citrus. a = Madeira Isl<strong>and</strong>. b = on lemon. c = in<br />
Southern Spain. d = only in Canary Isl<strong>and</strong>s. e = limited areas. f = North of Portugal. g = not reported in<br />
the main citrus growing areas of Spain yet. h = Azores. i = Algarve. j = on young trees. k = in<br />
nurseries. l = on m<strong>and</strong>arin. m = on sweet orange. n = natural enemies disruption. o = in western<br />
Andalusia. Ratings of species considered key-pests in at least one country are shown in bold.
CITRUS PEST MANAGEMENT IN THE MEDITERRANEAN BASIN 13<br />
Table 3. Visual inspection practices.<br />
Plant parts<br />
During the growing season/<br />
warm periods of the year<br />
Twigs<br />
Apical twigs of…<br />
Green twigs<br />
Previous flushing<br />
twigs<br />
Flowers<br />
Purpose – target pest<br />
Twigs are shaken <strong>by</strong> h<strong>and</strong> <strong>and</strong> the number of adults of<br />
whiteflies taking flight is noted (every week)<br />
Observations are made on the presence of honeydew,<br />
sooty mould <strong>and</strong> ants, which are associated with the<br />
presence of aphids, whiteflies <strong>and</strong> soft scales as well as<br />
on cottony egg masses which are associated with<br />
mealybugs. Parasitism should be also recorded<br />
Detection of the citrus leafminer<br />
Monitoring the presence of aphids (every week) <strong>and</strong><br />
Closterotomus trivialis (spring)<br />
Monitoring the development of armoured scales (every<br />
2 weeks), soft scales (every 2–3 weeks) <strong>and</strong> 1st <strong>and</strong> 2nd<br />
instar nymphs of Icerya purchasi<br />
Detection of Eriophyes sheldoni-affected <strong>org</strong>ans in<br />
spring <strong>and</strong> mid-summer<br />
Detection of the citrus moth<br />
Fruits Monitoring the development of diaspidid scales (every 2<br />
weeks) <strong>and</strong> locating foci of infestation<br />
Fruits <strong>and</strong> fruit stem inspections for mealybugs, white<br />
cottony egg mass, sooty mould developed on secreted<br />
honeydew <strong>and</strong> ants, which are associated with<br />
mealybugs (every 2 weeks)<br />
Detection of the citrus moth<br />
Detection of Tetranychus urticae during the summerearly<br />
autumn<br />
Detection of Ceratitis capitata as colour change begins<br />
In the packinghouse, presence of diaspidid scales should<br />
be checked<br />
Young leaves Detection of whitefly <strong>and</strong> soft scales foci of infestation<br />
in the orchard<br />
Observations are made on the presence of sooty mould<br />
<strong>and</strong> ants, which are associated with whiteflies, soft<br />
scales <strong>and</strong> mealybugs (every 2–3 weeks)<br />
Detection of the citrus mite, Panonychus citri, at the end<br />
of summer<br />
Cold periods of the year<br />
Twigs<br />
Detection of T. urticae from May to October<br />
Detection of 3rd instar nymphs <strong>and</strong> pre-ovipositing<br />
females of I. purchasi<br />
a Visual inspections also allow monitoring coccinellid predators on trees.
14<br />
J.A. JACAS ET AL.<br />
Table 4. Insect pests trapping methods.<br />
Type of trap<br />
Yellow water-pan traps<br />
Suction traps of 12 m high<br />
Yellow sticky traps<br />
Sex pheromone-baited traps<br />
White traps coated with glue mixed<br />
with trimedlure as well as other sex<br />
<strong>and</strong> food attractants<br />
Transparent sticky b<strong>and</strong> traps<br />
Beating branches of trees with a<br />
rubber-covered stick over a 1 m 2<br />
cloth screen<br />
Purpose – target pest<br />
Monitoring aphids: Moericke pan-traps, both square<br />
(60 × 60 × 10 cm) <strong>and</strong> round (30 cm in diameter),<br />
painted canary yellow inside <strong>and</strong> containing water<br />
with a spoonful of added detergent up to a depth of<br />
3–4 cm are commonly used; should be placed in the<br />
citrus orchards in mid-spring, 2–5 traps/ha, 70 cm<br />
above the ground, to be checked 1–2 times/week<br />
during the growing season<br />
Monitoring aphids<br />
Catching newly emerged whitefly adults: traps<br />
should be placed in the lower outside canopy of the<br />
south or southeast quadrant of the tree<br />
Catching males of Aonidiella aurantii <strong>and</strong> other<br />
armoured scales<br />
Monitoring parasitoids <strong>and</strong> detection of leafhoppers<br />
(Empoasca spp.)<br />
Attracting adult males of A. aurantii [pheromone (3Z,<br />
6R)-3-methyl-6-isopropenyl-3.9-decadien-l-yl<br />
acetate]; 2–5 traps/ha at 1.8–2.5 height above the<br />
ground, to be checked twice a week from early spring<br />
to mid-late autumn<br />
Attracting adult males of Planococcus citri: various<br />
designs of traps available, the yellow or white sticky<br />
trap with pheromone [(1R-CIS)-3-isopropenyl-2.2-<br />
dimethylcyclobutyl-methyl acetate] dispenser being<br />
most effective; 2–5 traps/ha; catches to be correlated<br />
with shifts in the population densities of female<br />
mealybugs<br />
Monitoring of the citrus moth, Prays citri<br />
Catching adults of Ceratitis capitata; 10 traps/ha<br />
Measuring the density of crawlers of A. aurantii in<br />
order to determine the timing of chemical treatment;<br />
the traps are tightly fixed around heavily infested<br />
twigs from mid spring onwards<br />
For other diaspidids <strong>and</strong> soft scales<br />
Monitoring coccinellid predators
CITRUS PEST MANAGEMENT IN THE MEDITERRANEAN BASIN 15
16<br />
J.A. JACAS ET AL.
CITRUS PEST MANAGEMENT IN THE MEDITERRANEAN BASIN 17
18<br />
J.A. JACAS ET AL.
CITRUS PEST MANAGEMENT IN THE MEDITERRANEAN BASIN 19
20<br />
J.A. JACAS ET AL.
2.3. Chemical Control<br />
CITRUS PEST MANAGEMENT IN THE MEDITERRANEAN BASIN 21<br />
Although many classical or augmentative biological control trials of arthropod pests<br />
have been successful in citrus, chemical control is still used. The recently finalized<br />
EU Review Programme on the inclusion of old active substances of plant protection<br />
products (registered in the EU up to 1993) in the positive list (Annex I) of the<br />
Directive 91/414/EEC (CEC, 1991), based on agreed <strong>and</strong> harmonised criteria for<br />
evaluating the safety of pesticides, resulted in a modification of the availability of<br />
insecticides, acaricides <strong>and</strong> insect attractants authorized for citrus pest management<br />
in the various member states of the E.U. (Tables 6 <strong>and</strong> 7) (Hellenic Ministry of<br />
Rural Development <strong>and</strong> Food, 2008; MAPA, 2008; MiPAAF, 2008). Some of these<br />
pesticides were also tested to evaluate their side effects on beneficial arthropods<br />
(Table 8).<br />
Table 6. Insecticides, acaricides <strong>and</strong> insect attractants (active substances) registered for use<br />
on citrus in Spain, <strong>Italy</strong> <strong>and</strong> Greece (June 2008).<br />
Country<br />
Spain<br />
<strong>Italy</strong><br />
Insecticides/acaricides/insect attractants (active substances)<br />
Abamectin (O, L, M, G), acetamiprid (O, L, M, G), alpha-cypermethrin<br />
(O, L, M, G), azadirachtin (O, L, M, G), Bacillus thuringiensis var.<br />
kurstaki (O, L, M, G), benfuracarb (O, L, M, G), bifentrin (O, L, M,<br />
G), buprofezin (O, L, M, G), carbosulfan (O, L, M, G), chlorpyrifos<br />
(O, L, M, G), chlorpyrifos-methyl (O, L, M), cihexatin (O, L, M, G),<br />
clofentezine (O,L,M,G), cypermethrin (O, L, M, G), deltamethrin (O,<br />
L, M, G), diazinon (O, L, M, G), dichlorvos (O, L, M, G), dicofol (O,<br />
L, M, G), diflubenzuron (O, M, G), dimethoate (O, L, M, G),<br />
etofenprox (O, M, G), etoxazol (O, M), fenazaquin (O, M, G),<br />
fenbutatin oxide (O, M, G), fenitrothion (O, L, M, G), fenoxycarb (O,<br />
M, G), fenpyroximate (O, L, M, G), flufenoxuron (O, M, G),<br />
hexythiazox (O, L, M, G), imidacloprid (O, L, M, G), kaolin (O, M),<br />
lambda-cyhalothrin (O, L, M, G), lufenuron (O, L, M, G), malathion<br />
(O, L, M, G), methomyl (O, L, M, G), methoxyfenozide (O, M),<br />
mineral oil (O, L, M, G), oxydemeton-methyl (O, L, M, G), phosmet<br />
(O, L, M, G), piridaben (O, L, M, G), pirimicarb (O, L, M, G),<br />
pirimiphos-methyl (O, L, M, G), potassium salts of vegetable fatty<br />
acids (O, L, M), propargite (O, L, M, G), pymetrozine (O, L, M, G),<br />
pyriproxifen (O, L, M, G), spinosad (O, L, M, G), tau-fluvalinate (O,<br />
L, M, G), tebufenozide (O, L, M, G), tebufenpyrad (O, L, M, G),<br />
trichlorfon (O, L, M, G)<br />
Abamectin (O, L, M), acrinathrin (O, L, G), alfamethrin (O, L, M),<br />
azadirachtin (O, L, M, G), Bacillus thurigiensis var. aizawai (O, L, M),<br />
Bacillus thurigiensis var. kurstaki (O, L, M), Beauveria bassiana (O,<br />
L, M), bifentrin (O, L, M), buprofezin (O, L, M), calcium polysulfur
22<br />
J.A. JACAS ET AL.<br />
Table 6 continued<br />
Greece<br />
(O, L, M), chlorpyrifos (O, L, M), chlorpyrifos-methyl (O, L, M, C),<br />
clofentezine (O, L, M, Cl, G, B), cypermethrin (O, L), deltamethrin (O,<br />
L, M), diazinon (O) (1), dicofol (O, L, M), dimethoate (O, L, M) (2),<br />
ethoprophos (O, L, M), etofenprox (O, L, M, Cl, B, SO, G, P, T, C),<br />
etoxazol (O, L, M, Cl, B, SO, G, P, T, C), fenazaquin (O, L, M, Cl),<br />
fenbutatin oxide (O, L, M), fenpyroximate (O, L, Cl), flufenoxuron (O,<br />
M, Cl), fluvalinate (O, M), hexythiazox (O, L, M), imidacloprid (O, L,<br />
M, Cl), lambda-cyhalothrin (O), lufenuron (O, L, M, Cl), malathion<br />
(O, L, M, Cl, B, SO, G, P, T, C) (1), methomyl (O, L, M),<br />
methoxyfenozide (O, M, Cl), mineral oil (O, L, M, Cl), phosalone (O,<br />
L, M) (3), phosmet (O, L, M), pirimicarb (O, L, M), pirimiphos-methyl<br />
(O, L), propargite (O, L, M, G, Cl), pymetrozine (O, L, M, Cl),<br />
pyrethrines (O, L, M), pyridaben (O, L, M, Cl, T), pyriproxifen (O, L,<br />
M), rotenone (O, L, M), spinosad (as bait) (O, L, M, Cl, SO, C, G, B,<br />
T), spirodiclofen (O, L, M, Cl, G, B, C, SO), tebufenozide (O, L, M),<br />
tebufenpyrad (O, L, M, Cl, G, C, T, B), thiamethoxam (O, L, M, Cl),<br />
trichlorfon (O, L, M) (4), zeta-cypermethrin (O, L)<br />
Acetamiprid (O, L, M, <strong>and</strong> nurseries, G, C), azadirachtin (O, L, M, G),<br />
Bacillus thurigiensis var. aizawai (O, L, M, G, C), Bacillus<br />
thuringiensis var. kurstaki (O, L, M, G, C), Beauveria bassiana (M),<br />
buprofezin (O, L, M, G, SO, C), chlorpyrifos (O, L, M, G, P),<br />
chlorpyrifos-methyl (O, L, M), cypermethrin (O, M,G), deltamethrin<br />
(O, L, M, G, C, P), diflubenzuron (O, L, M, G, P), fatty acid potassium<br />
salt (O, L, M, G, C), fenoxycarb (O, L, M), flucythrinate (O, L, M, G),<br />
flufenoxuron (O, L), imidacloprid (O, L, M, G), methomyl (O, L, M,<br />
P), methoxyfenozide (O, M, G), mineral oil (O, L, M, G, SO, P),<br />
phosmet (O, L, M, G), pirimicarb (O, L, M, G, P), pymetrozine (O),<br />
pirimiphos-methyl (M), pyrethrins (O, L, M, G), pyriproxyfen (O, L,<br />
M), tau-fluvalinate (O, L, M, G), tebufenozide (L, M), thiamethoxam<br />
(O, L, M)<br />
Insect attractants: farnesol (O, L, M, G), nerolidol (O, L, M, G)<br />
O: Orange, L: Lemon, M: M<strong>and</strong>arin, G: Grapefruit, SO: Sour orange, C: Citron, P: Pomelo, Cl:<br />
Clementine, T: Tangerine, B: Bergamot. 1 = Active substance not included in the Annex I of the<br />
directive 91/414/EC, the commercial plant production products are revoked from 6 December 2007<br />
<strong>and</strong> the stocks were commercialized <strong>and</strong> used until 6 December 2008. 2 = Use allowed only on<br />
nonproductive orchards. For some commercial plant production products the extension of the<br />
authorization for use on citrus to control aphids has been approved with a pre-harvest interval of 100<br />
days. 3 = Active substance not included in the Annex I of the directive 91/414/EC. The<br />
authorization of the commercial plant production products containing phosalone is revoked from 23<br />
June 2007. The stocks were commercialized <strong>and</strong> used until 22 June 2008. 4 = Active substance not<br />
included in the Annex I of the directive 91/414/EC. The authorization of the commercial plant<br />
production products containing this a.i. is revoked from 21 November 2007. The stocks were<br />
commercialized <strong>and</strong> used until 21 November 2008.
CITRUS PEST MANAGEMENT IN THE MEDITERRANEAN BASIN 23<br />
Table 7. Insecticides, acaricides <strong>and</strong> insect attractants (active substances) registered for use<br />
against the main arthropod pests of citrus in Spain, <strong>Italy</strong> <strong>and</strong> Greece (June 2008).<br />
Pest<br />
Thrips (Thysanoptera)<br />
Whiteflies (Aleyrodidae)<br />
Aleurothrixus floccosus<br />
Dialeurodes citri<br />
Aphids (Aphididae)<br />
Aphis gossypii<br />
Aphis spiraecola<br />
Toxoptera aurantii<br />
Toxoptera citricida<br />
Armoured scales (Diaspididae)<br />
Aonidiella aurantii<br />
Aspidiotus nerii<br />
Chrysomphalus dityospermi<br />
Lepidosaphes beckii<br />
Parlatoria perg<strong>and</strong>ei<br />
Parlatoria ziziphi<br />
Unaspis citri<br />
Soft scales (Coccidae)<br />
Ceroplastes sinensis<br />
Coccus hesperidum<br />
Saissetia oleae<br />
Insecticides/acaricides (active substance) a<br />
Acrinathrin (I), chlorpyrifos (G), fatty acid potassium salt<br />
(G), malathion (I), pirimiphos-methyl (I), rotenone (I)<br />
Acetamiprid (S), azadirachtin (S, G), buprofezin (S, G),<br />
carbosulfan (S), chlorpyrifos (S), cypermethrin (I),<br />
deltamethrin (I), dimethoate (S), etofenprox (S), fatty acid<br />
potassium salt (G), fenazaquin (S, I), fenpyroximate (S),<br />
imidacloprid (S, I, G), lufenuron (S, I), malathion (S, I),<br />
methomyl (S), mineral oil (G), phosmet (S), piridaben (S),<br />
pyrimiphos-methyl (S), rotenone (I), zeta-cypermethrin (I)<br />
Acetamiprid (S, G), alpha-cypermethrin (S), azadirachtin<br />
(S, G), benfuracarb (S), bifentrin (S), carbosulfan (S),<br />
chlorpyrifos (S, G), chlorpyrifos-methyl (G),<br />
cypermethrin (S, I, G), deltamethrin (S, I), dimethoate (S),<br />
etofenprox (S), fatty acid potassium salt (G), fenitrothion<br />
(S), flucythrinate (G), fluvalinate (I), imidacloprid (S, I),<br />
lambda-cyhalothrin (I), malathion (I), methomyl (S),<br />
mineral oil (S, G), oxamyl (G), oxydemeton-methyl (S),<br />
phosmet (S), pimetrozine (S, I), pirimicarb (S, I,G),<br />
pyrimiphos-methyl (S, I), potassium salts of vegetable<br />
fatty acids (S), pymetrozine (G), pyrethrines (G), rotenone<br />
(I), tau-fluvalinate (S), thiamethoxam (I, G), zetacypermethrin<br />
(I)<br />
Azadirachtin (S), buprofezin (S, G), chlorpyrifos (S, G),<br />
chlorpyrifos-methyl (G), cypermethrin (I, G),<br />
flucythrinate (G), dimethoate (S), fenitrothion (S),<br />
fenoxycarb (S), fenpyroximate (S), malathion (S, I),<br />
methomyl (S, I), mineral oil (S, I, G), phosmet (S, I, G),<br />
pyrimiphos-methyl (S), pyriproxifen (S, I, G), rotenone (I)<br />
Azadirachtin (S), buprofezin (S), chlorpyrifos (S, G),<br />
chlorpyrifos-methyl (G), cypermethrin (S, I, G),<br />
deltamethrin (I), dimethoate (S), fenitrothion (S),<br />
fenoxycarb (S, G), fenpyroximate (S), flucythrinate (G),<br />
imidacloprid malathion (S), malathion (I), methomyl (S,<br />
I), mineral oil (S, I, G), phosmet (S, I), pyriproxifen (S, I,<br />
G), pyrimiphos-methyl (S), rotenone (I), tau-fluvalinate<br />
(S)
24<br />
J.A. JACAS ET AL.<br />
Table 7 continued<br />
Mealybugs (Pseudococcidae)<br />
Planococcus citri<br />
Moths<br />
Phyllocnistis citrella<br />
(Gracillariidae)<br />
Prays citri (Hyponomeutidae)<br />
Fruit flies (Tephritidae)<br />
Ceratitis capitata<br />
Mites<br />
Eutetranychus banksi<br />
Panonychus citri<br />
Phyllocoptruta oleivora<br />
Tetranychus urticae<br />
Azadirachtin (S), buprofezin (S, G), chlorpyrifos (S, G),<br />
cypermethrin (I, G), dimethoate (S), fenitrothion (S),<br />
flucythrinate (G), malathion (S, I), methomyl (S, I),<br />
mineral oil (S, I, G), phosmet (S, I, G), pyrimiphos-methyl<br />
(S, I), rotenone (I)<br />
Abamectin (S, I: P. citrella), acetamiprid (G: P. citrella<br />
nurseries), alpha-cypermethrin (S), azadirachtin (S, G: P.<br />
citrella), Bacillus thuringiensis var. aizawai (G: P. citri),<br />
Bacillus thuringiensis var. kurstaki (S, G: P. citri),<br />
benfuracarb (S), buprofezin (P. citrella), carbosulfan (S),<br />
chlorpyrifos (S, G), cypermethrin (S, I: P. citri, G),<br />
deltamethrin (S), diazinon (S), dichlorvos (S),<br />
diflubenzuron (S) dimethoate (S), etofenprox (S),<br />
fenitrothion (S), fenoxycarb (S), fenpyroximate (S),<br />
flucythrinate (G: P. citri), flufenoxuron (S, I, G: P.<br />
citrella), imidacloprid (S, I, G: P. citrella), lufenuron (S,<br />
I), malathion (S, I), methomyl (S, I), methoxyfenozide (I,<br />
G: P. citrella), mineral oil (G), phosmet (S, I),<br />
pyrimiphos-methyl (S, I), rotenone (I: P. citri) taufluvalinate<br />
(S), tebufenozide (S, I, G: P. citrella),<br />
thiamethoxam (I, G: P. citrella)<br />
Azadirachtin (S), Beauveria bassiana (G), cypermethrin<br />
(I, G), deltamethrin (I), dichlorvos (S), etofenprox (I),<br />
flucythrinate (G), imidacloprid (S), lambda-cyhalothrin<br />
(S, I), lufenuron (S), malathion (S, I), phosmet (S, I, G),<br />
pyrimiphos-methyl (I), rotenone (I), spinosad bait (I),<br />
trichlorfon (S, I), zeta-cypermethrin (I)<br />
Abamectin (S, I: T. urticae), acrinathrin (I), bifentrin (S),<br />
buprofezin (S), clofentezine (S, I), dicofol (S, I, G),<br />
etoxazol (S, I, G), fenazaquin (S, I, G), fenbutatin oxide<br />
(S, I, G), fenitrothion (S), fenpyroximate (S, I),<br />
flufenoxuron (S, I), hexythiazox (S, I), malathion (S),<br />
mineral oil (S, I, G), oxamyl (G), oxydemeton-methyl (S),<br />
propargite (S, I, G), pyridaben (S, I), pyrimiphos-methyl<br />
(S, I), spirodiclofen (I), tebufenpyrad (S, I, G)<br />
a<br />
G = Greece; I = <strong>Italy</strong>; S = Spain.
CITRUS PEST MANAGEMENT IN THE MEDITERRANEAN BASIN 25<br />
Table 8. Side effects of pesticides (active substances ), registered for the control of citrus<br />
a<br />
pests, on beneficial arthropods .<br />
Active substance<br />
Rodolia<br />
cardinalis<br />
Cryptolaemus<br />
montrouzieri<br />
Euseius<br />
stipulatus<br />
Lysiphlebus<br />
testaceipes<br />
Leptomastix<br />
dactylopii<br />
Cales noacki<br />
Abamectin 1 3–4 2–3 3–4<br />
Azadirachtin 3–4 1 1 1 3–4<br />
Bacillus thuringiensis<br />
var. kusrtaki<br />
1 1 1 1 1 1<br />
Benfuracarb 1 2–3<br />
Bifentrin 3–4 3–4 1<br />
Buprofezin 1–2 3 1–2 1 1–2 1<br />
Carbosulfan 1–2 1–2 1 2–3<br />
Chlorpyrifos 1–2 2 2 3 3 2–3<br />
Chlorpyrifos-methyl 1 1 3 3 2–4 1–2<br />
Clofentezine 1 2 1–2 1<br />
Cypermethrin 4 4 4 1 3–4<br />
Deltamethrin 4 3–4 4 1 4 3<br />
Diazinon 3 2 3 1–2<br />
Dicofol 1 1–4 3–4 1 3–4 2<br />
Diflubenzuron 1 1–2<br />
Dimethoate 1 4 2–3 1–2 4 2<br />
Fenazaquin 4 2 4 3<br />
Fenbutatin oxide 1 2 1 1 1<br />
Fenitrothion 1–2 3 1–2 4 3<br />
Fenoxycarb 4 1–2 2<br />
Flucythrinate 2 3<br />
Flufenoxuron 2–3 1–2<br />
Fosalone 2 1 3<br />
Hexythiazox 1 1 1<br />
Imidacloprid 4 2–3 1 4 3<br />
Lambda-cyhalothrin 3<br />
Lufenuron 4 1 1 1<br />
Malathion 2–3 4 2 3 4 3–4<br />
Methomyl 4 4 4 2 3–4<br />
Mineral oil 1 1–2 1–2 2 1 1–4<br />
Oxydemeton-methyl 1 3 2 1 3 1–2<br />
Phosmet 4 4 2–3 1 3 4<br />
Piridaben 4 1<br />
Pirimicarb 1–2 2 1–2 1 1 1<br />
Pyrimiphos-methyl 1–2 1–2 1–4 4 3–4<br />
Propargite 4 1 2–3<br />
Pyriproxifen 4 4 1 1–2 2–3<br />
Spinosad 1 1 4 3–4
26<br />
J.A. JACAS ET AL.<br />
Table 8 continued<br />
Tau-fluvalinate 4 3 3–4 1 3 2<br />
Tebufenozide 1<br />
Tebufenpyrad 2<br />
Trichlorfon 2–3 1 1 3 1–2 2<br />
Zeta-cypermethrin 4 4 4 1 3–4<br />
a Classification according to the IOBC WG “Pesticides <strong>and</strong> Beneficial Organisms” st<strong>and</strong>ards: 1 =<br />
harmless; 2 = slightly harmful; 3 = moderately harmful; 4 = harmful (sources: Jacas & García Marí, 2001;<br />
Pascual-Ruíz & Urbaneja, 2006; Urbaneja et al., 2008; Suma, Zappalà, Mazzeo, & Siscaro, 2009).<br />
REFERENCES<br />
Amaro, P. (1992). História da luta biológica em Portugal. Revista de Ciências Agrárias, 15, 31–47.<br />
Beardsley, J. W., AliNiazee, M. T. & Watson, T. F. (1979). Sampling <strong>and</strong> monitoring. In D. W. Davis,<br />
S. C. Hoyt, J. A. McMurty, & M. T. AliNiazee (Eds.), Biological control <strong>and</strong> insect pest<br />
management (pp. 11–22). California: University of California, Division of Agricultural Sciences.<br />
Cavalloro, R., & Prota R. (Eds.) (1983). Proceedings of the E.C. Experts’ Meeting Integrated Control in<br />
Citrus: Comparison of results achieved <strong>by</strong> applying a st<strong>and</strong>ardized methodology (pp. 39–42).<br />
Siniscola-Muravera, 20–22 October 1982.<br />
CEC [Council of the European Communities]. (1991). Council directive of 15 July 1991 concerning the<br />
placing of plant protection products on the market. http://europa.eu/eur-lex/en/consleg/pdf/1991/<br />
en_1991L0414_do_001.pdf<br />
De Bach, P. (1964). Biological control of insect pests <strong>and</strong> weeds. London: Chapman <strong>and</strong> Hall Ltd.<br />
El-Otmani M., Srairi I., & Benhaddou, A. (2007). National citrus sector analysis: Morocco.<br />
Euromedcitrusnet Project, Deliverable 9. The European Union 6th Framework Programme, food<br />
quality <strong>and</strong> safety. Available at: http://www2.spi.pt/euromedcitrusnet/Documents/Sector%20-<br />
Analysis%20Report/EuroMedCitrusNet%20Sector%20Analysis%20Report-Morocco.pdf<br />
EPPO [European <strong>and</strong> Mediterranean Plant Protection Organization]. (2007). EPPO A1 <strong>and</strong> A2 lists of<br />
pests recommended for regulation as quarantine pests. September 2007. Available at:<br />
http://archives.eppo.<strong>org</strong>/EPPOSt<strong>and</strong>ards/PM1_GENERAL/pm1-02(16)_A1A2_2007.pdf<br />
Franco, J. C., García-Marí, F., Ramos, A. P., & Besri, M. (2006). Survey on the situation of citrus pest<br />
management in Mediterranean countries. IOBC/wprs Bulletin, 29(3), 335–346.<br />
Gomes da Silva, R., B<strong>org</strong>es da Silva, E., & Franco, J. C. (2006). Parasitoid complex of citrus leafminer<br />
on lemon orchards in Portugal. IOBC/wprs Bulletin, 29(3), 197–204.<br />
Hellenic Ministry of Rural Development <strong>and</strong> Food. (2008). Authorized plant protection products data<br />
base. http://www.minagric.gr/syspest/<br />
IOBC/WPRS Commission “IP Guidelines <strong>and</strong> Endorsement”. (2004). Guidelines for integrated<br />
production of citrus. http://www.iobc.ch/IOBC_Citrusguideline_english_definitive.pdf<br />
ISTAT [Istituto Nazionale di Statistica]. (2007). Dati annuali sulle coltivazioni. Available at:<br />
http://www.istat.it/agricoltura/datiagri/coltivazioni/anno2007/ital2007.htm<br />
Jacas, J. A., & García-Marí, F. (2001). Side-effects of pesticides on selected natural enemies occurring in<br />
citrus in Spain. IOBC/wprs Bulletin, 24, 103–112.<br />
Jacas, J. A., Urbaneja, A., & Viñuela, E. (2006). History <strong>and</strong> future of introduction of exotic arthropod<br />
biological control agents in Spain: A dilemma? BioControl, 51, 1–30.<br />
Kalaitzaki, A. P., (2004). Study of biological parameters of parasitoids of Phyllocnists citrella Stainton<br />
<strong>and</strong> their impact on the dynamic of its population. PhD Thesis, Agricultural University of Athens.<br />
Katsoyannos, P. (1996). Integrated insect pest management for citrus in northern Mediterranean<br />
countries. Benaki Phytopathological Institute, Athens, Greece.<br />
Laajimi, A., & Ben Mimoun, M. (2007). National citrus sector analysis: Tunisia. Euromedcitrusnet<br />
Project, Deliverable 9. The European Union 6th Framework Programme, Food Quality <strong>and</strong> Safety.<br />
http://www2.spi.pt/euromedcitrusnet/Documents/Sector%20Analysis%20Report/EuroMedCitrusNet<br />
%20Sector%20Analysis%20Report-Tunisia.pdf
CITRUS PEST MANAGEMENT IN THE MEDITERRANEAN BASIN 27<br />
Malausa, J. C., Rabasse, J. M., & Kreiter, P. (2008). Les insectes entomophages d’intérêt agricole acclimatés<br />
en France métropolitaine depuis le début du 20 ème siècle. Bulletin OEPP/EPPO, 38, 136–146.<br />
MAPA [Ministerio de Agricultura, Pesca y Alimentación]. (2007). Anuario de Estadística Agraria.<br />
Madrid, Spain.<br />
MAPA. (2008). Registro de productos fitosanitarios. http://www.mapa.es/es/agricultura/pags/fitos/<br />
registro/menu.asp<br />
MiPAAF [Ministero delle Politiche Agricole, Alimentari e Forestali]. (2008). Banca Dati Fitofarmaci.<br />
Centro di Ricerca per la Patologia Vegetale, Roma. http://www.sian.it/fitovis/<br />
Noyes, J. S., & Hayat, M. (1994). Oriental parasitoids of the Anagyrini (Hymenoptera: Encyrtidae).<br />
Oxon, UK: CAB International.<br />
Pascual-Ruiz, S., & Urbaneja, A. (2006). Lista de Efectos Secundarios de Plaguicidas sobre Fauna Útil en<br />
Cítricos. Levante Agrícola, 380, 186–191.<br />
Salama Eid, S. S, Latif, F., & Hassan E. (2007). National Citrus Sector Analysis. Euromedcitrusnet.<br />
Project, Deliverable 9. The European Union 6th Framework Programme, food quality <strong>and</strong> safety.<br />
Available at: http://www2.spi.pt/euromedcitrusnet/Documents/Sector%20Analysis%20Report/Euro-<br />
MedCitrusNet%20Sector%20Analysis%20Report%20-Egypt.pdf<br />
Siscaro, G., Caleca, V., Reina, P., Rizzo, M. C., & Zappalà, L. (2003). Current status of the biological<br />
control of the citrus leafminer in Sicily. IOBC/WPRS Bulletin, 26(6), 29–36.<br />
Siscaro, G., Di Franco, F., & Zappalà, L. (2008). On the presence <strong>and</strong> diffusion of Comperiella bifasciata<br />
How. (Hymenoptera: Encyrtidae) in Southern <strong>Italy</strong>. IOBC/wprs Bulletin, 38, 42–45.<br />
Suma, P., Zappalà, L., Mazzeo, G., & Siscaro, G. (2009). Lethal <strong>and</strong> sublethal effects of insecticides on<br />
natural enemies of citrus scale pests. BioControl, 54, 651–661.<br />
Tsagarakis, A., Kalaitzaki, A. P., Lykouressis, D., Michelakis, S., & Alex<strong>and</strong>rakis V. (1999). Presence<br />
<strong>and</strong> impact of introduced <strong>and</strong> native parasitoids on Phyllocnists citrella Stainton in Greece.<br />
Evaluating indirect ecological effects of biological control, global IOBC International Symposium,<br />
Montpellier, France, 17–20 October 1999. IOBC/wprs Bulletin, 22, 66.<br />
Urbaneja, A., Pascual Ruiz, S., Pina, T., Abad-Moyano, R., Vanaclocha, P., Montón, H., et al. (2008).<br />
Efficacy of five selected acaricides against Tetranychus urticae (Acari: Tetranychidae) <strong>and</strong> their<br />
side effects on relevant natural enemies occurring in citrus orchards. Pest Management Science, 64,<br />
834–842.<br />
Viggiani, G. (1975). La lotta biologica di tipo convenzionale. Atti del X Congresso Nazionale Italiano di<br />
Entomologia (pp. 161–187), Sassari 20–25 maggio 1974.<br />
Zappalà, L., Siscaro, G., & Longo, S. (2008). Establishment of Neodryinus typhlocybae (Ashmead)<br />
(Hymenoptera: Dryinidae) in Sicilian lemon orchards. IOBC/wprs Bulletin, 38, 280–283.
2<br />
MAIN ARTHROPOD PESTS OF CITRUS CULTURE<br />
AND PEST MANAGEMENT IN GREECE<br />
§<br />
FILITSA KARAMAOUNA, PANAGIOTIS MYLONAS,<br />
DIMITRIOS PAPACHRISTOS, DIMITRIOS KONTODIMAS,<br />
ANTONIOS MICHAELAKIS AND ELEFTHERIA KAPAXIDI<br />
Benaki Phytopathological Institute,<br />
145 61 Kifissia, Greece<br />
Abstract. The key arthropod pests in the citrus producing areas in Greece comprise the Mediterranean<br />
fruit fly Ceratitis capitata, the California red scale Aonidiella aurantii <strong>and</strong> the citrus mealybug<br />
Planococcus citri. Outbreaks of the whiteflies Aleurothrixus floccosus <strong>and</strong> Dialeurodes citri, the scales<br />
Ceroplastes rusci <strong>and</strong> Saissetia oleae as well as the Tetranychidae mites Panonychus citri <strong>and</strong><br />
Tetranychus urticae <strong>and</strong> the Eriophyiidae mites Aculops pelekassi <strong>and</strong> Aceria sheldoni may occur<br />
locally. The citrus leafminer Phyllocnistis citrella, aphids (Aphis spiraecola, A. gossypii, Toxoptera<br />
aurantii) <strong>and</strong> thrips (Heliothrips haemorrhoidalis, Pezothrips kellyanus) are of minor importance. The<br />
problems due to major <strong>and</strong> minor citrus pests <strong>and</strong> control measures in Greece are reviewed <strong>and</strong><br />
Integrated Pest Management (IPM) strategies are recommended.<br />
1. INTRODUCTION<br />
The total citrus-producing area in Greece is 57,525.6 hectares (ha). The most<br />
widely cultivated Citrus species include orange Citrus sinensis (L.) Osbeck<br />
(40,054 ha), lemon Citrus limon Burman f. (10,497 ha), m<strong>and</strong>arin Citrus reticulata<br />
Blanco (6,514 ha), grapefruit Citrus paradisi Macfadyen (340 ha), citron Citrus<br />
medica L. (100 ha), bergamot Citrus bergamia Risso (12 ha), bitter orange Citrus<br />
aurantium L. (7.82 ha) <strong>and</strong> pumelo Citrus maxima (Burm) Merrill (0.78 ha)<br />
(Hellenic Ministry of Rural Development <strong>and</strong> Food, 2006, Unpublished data).<br />
Major arthropod pests in terms of importance in the citrus-growing regions of the<br />
country comprise the Mediterranean fruit fly Ceratitis capitata (Wiedemann)<br />
(Diptera: Tephritidae), the California red scale Aonidiella aurantii (Maskell)<br />
(Hemiptera: Diaspididae) <strong>and</strong> the mealybug Planococcus citri (Risso) (Hemiptera:<br />
Pseudococcidae). However, outbreaks of the woolly whitefly Aleurothrixus<br />
floccosus Maskell (Hemiptera: Aleyrodidae), the citrus whitefly Dialeurodes citri<br />
§All authors contributed equally to this chapter.<br />
A. <strong>Ciancio</strong>, K.G. Mukerji (eds.), Integrated Management of Arthropod Pests<br />
<strong>and</strong> Insect Borne Diseases, Integrated Management of Plant Pests <strong>and</strong> Diseases 5,<br />
DOI 10.1007/978-90-481-8606-8_2, © Springer Science+Business Media B.V. 2010<br />
29
30<br />
F. KARAMAOUNA ET AL.<br />
(Ashmead) (Hemiptera: Aleyrodidae), Ceroplastes rusci L (Hemiptera: Coccidae),<br />
the Mediterranean black scale Saissetia oleae (Bernard) (Hemiptera: Coccidae) <strong>and</strong><br />
Tetranychidae <strong>and</strong> Eriophyiidae mites are recorded at small (local) scale. The<br />
citrus leafminer Phyllocnistis citrella (Stainton) (Lepidoptera: Gracillariidae) <strong>and</strong><br />
the citrus infesting aphids <strong>and</strong> thrips are of minor importance (Hellenic Ministry of<br />
Rural Development <strong>and</strong> Food <strong>and</strong> Regional Plant Protection Services, 2007,<br />
unpublished data).<br />
2. PEST STATUS AND CONTROL MEASURES<br />
An idea for the present status of the citrus arthropod pests in the citrus-producing<br />
areas of Greece can be obtained from an empirical risk assessment of the Hellenic<br />
Ministry of Rural Development <strong>and</strong> Food, which is based on data from the<br />
Regional Plant Protection Services of the Ministry (2007). A rank scale from 1 to 3<br />
is used (1 being the most serious pest to 3 being the less serious one) so that the<br />
citrus arthropod pest status is as follows: the Mediterranean fruit fly Ceratitis<br />
capitata (1–2); the California red scale Aonidiella aurantii (1–3); the mealybug<br />
Planococcus citri (1–3); the woolly whitefly Aleurothrixus floccosus (1–3); the<br />
citrus whitefly Dialeurodes citri (Ashmead) (Hemiptera: Aleyrodidae) (1) locally<br />
on the isl<strong>and</strong> of Crete; Ceroplastes rusci (1) locally in Argolis-Peloponnese; the<br />
Mediterranean black scale Saissetia oleae (1) locally in Argolis; the Tetranychidae<br />
mites Panonychus citri <strong>and</strong> Tetranychus urticae (1–3) locally in Peloponnese; the<br />
Eriophyiidae mites Aculops pelekassi <strong>and</strong> Aceria sheldoni (1–3) locally in Argolis–<br />
Peloponnese <strong>and</strong> the western mainl<strong>and</strong>; the citrus flower moth Prays citri Milliére<br />
(Lepidoptera: Hyponomeutidae) (2); the purple scale Lepidosaphes beckii<br />
(Newman) (Hemiptera: Diaspididae) (2) locally in Argolis; the rose tortrix moth<br />
Archips rosanus (Lepidoptera: Tortricidae) locally in Argolis; the citrus leafminer<br />
Phyllocnistis citrella (2–3); Citrus infesting aphids (2–3) <strong>and</strong> thrips (3) locally in<br />
Achaia-Peloponnese (Hellenic Ministry of Rural Development <strong>and</strong> Food <strong>and</strong><br />
Regional Plant Protection Services, 2007, unpublished data).<br />
A forecasting/warning system concerning infestation <strong>by</strong> the main insect pests of<br />
the most important crops in the country, including Citrus, operates <strong>by</strong> the Regional<br />
Plant Protection Services of the Hellenic Ministry of Rural Development <strong>and</strong> Food.<br />
Forecasting of infestation is based on meteorological data, monitoring <strong>by</strong> trapping<br />
or sampling, historical <strong>and</strong> other data sources (literature, agronomists/consultants/<br />
farmers files). Instructions for preventive plant protection measures are provided to<br />
the citrus growers when there is an issue of warning (Table 1).<br />
A review of the problems <strong>and</strong> the control measures for the main citrus arthropod<br />
pests in Greece i.e. the Mediterranean fruit fly Ceratitis capitata, scale insects<br />
(especially A. aurantii <strong>and</strong> P. citri), whiteflies (especially A. floccossus), the citrus<br />
leafminer P. citrella, aphids, the citrus flower moth P. citri, thrips <strong>and</strong> mites will<br />
be presented in the following sections.
IPM OF CITRUS PESTS IN GREECE<br />
31<br />
Table 1. Citrus arthropod pests for which plant protection instructions are provided <strong>by</strong> the<br />
Regional Plant Protection Services in conventional citrus culture in Greece.<br />
Arthropod pest Meteo data Monitoring <strong>by</strong><br />
trapping/<br />
sampling<br />
Historical<br />
data<br />
Other data a<br />
Ceratitis capitata Y Y/Y Y Crete: Lit, A, F<br />
Aonidiella aurantii Y Y/Y Y Achaia: Population<br />
Prediction Model<br />
Crete: Lit, A, F<br />
Planococcus citri Y Y/Y Y Achaia: Population<br />
Prediction Model<br />
Crete: Lit, A, F<br />
Aleurothrixus<br />
floccosus<br />
N except<br />
Crete<br />
N/Y<br />
Y in most<br />
areas<br />
Crete: Lit, A, F<br />
Dialeurodes citri a Y N/Y Y Crete: Lit, A, F<br />
Ceroplastes rusci a N N/Y Y N<br />
Saissetia oleae a N N/Y Y N<br />
Mites<br />
Ν except<br />
Argolis<br />
N/Y N except<br />
Argolis<br />
N<br />
Prays citri<br />
Y in some<br />
areas<br />
Y in some<br />
areas/Y<br />
Lepidosaphes<br />
Y N/Y Y N<br />
beckii a<br />
Citrus aphids<br />
Phyllocnistis citrella<br />
N except<br />
Crete<br />
N except<br />
Crete<br />
N/Y<br />
N/Y<br />
Y<br />
Ν except<br />
Crete<br />
Y in some<br />
areas<br />
N<br />
Crete: Lit, A, F<br />
Crete: Lit, A, F<br />
Thrips b N N/Y N N<br />
a Y = Yes; N = No; Lit = Literature, A = Agronomists, F = Farmers. Source: Hellenic Ministry of Rural<br />
Development <strong>and</strong> Food <strong>and</strong> Regional Plant Protection Services (2006).<br />
b The pests cause problems in certain regions <strong>and</strong> data refer to those regions.<br />
2.1. The Mediterranean Fruit Fly, Ceratitis capitata<br />
The Mediterranean fruit fly (medfly) Ceratitis capitata was first recorded in<br />
Greece <strong>by</strong> Papage<strong>org</strong>iou in 1915 on infested citrus orchards in Attica <strong>and</strong> on the<br />
isl<strong>and</strong> of Aegina. Until today the presence of the medfly is reported almost all over<br />
Greece, except the highl<strong>and</strong>s of the continental country <strong>and</strong> the lowl<strong>and</strong> of the<br />
northwestern region. It infests mainly citrus fruits, pears, apples, peaches, apricots<br />
<strong>and</strong> figs <strong>and</strong> can cause serious yield losses (Tzimos, 1961; Mourikis, 1965;
32<br />
F. KARAMAOUNA ET AL.<br />
Michelakis, 1992; Zervas, Kateva, & Christopoulos, 1995; Papadopoulos &<br />
Economopoulos, 1997a; Katsoyannos, Kouloussis & Carey, 1998; Papadopoulos,<br />
1999; Papachristos, 2007).<br />
Adults of medfly are active from late spring until early winter <strong>and</strong> they are very<br />
abundant from the beginning of August until the end of October; they remain<br />
inactive or below detectable levels throughout the rest of the year (Zervas et al.,<br />
1995; Katsoyannos et al., 1998; Papadopoulos, 1999; Papachristos, 2007).<br />
However, in the southern part of the country (the isl<strong>and</strong> of Crete) the adults are<br />
active during winter (Mavrikakis, Economopoulos, & Carey, 2000). Larvae inside<br />
the infested fruits <strong>and</strong> pupae in the soil are the main stages of overwintering in the<br />
north whereas in Crete it appears that the medfly overwinters in all development<br />
stages (Mourikis, 1965; Zervas et al., 1995; Papadopoulos, Carey, Katsoyannos, &<br />
Kouloussis, 1996; Katsoyannos et al., 1998; Papadopoulos, 1999; Mavrikakis<br />
et al., 2000). Moreover, patterns of fluctuation of adult population size may be<br />
varying significantly even in the same region depending on the host plant<br />
composition <strong>and</strong> availability (Katsoyannos et al., 1998). Although the precise<br />
determination of C. capitata generations is difficult because of a high overlapping<br />
between them, it is considered that C. capitata completes 5–7 generations<br />
depending on the region <strong>and</strong> the year (Mourikis, 1965).<br />
Infestation of citrus fruits starts as soon as they begin to ripen <strong>and</strong> continues until<br />
they are completely ripe. Among the main citrus species, the most susceptible one is<br />
bitter orange, followed <strong>by</strong> orange, whereas lemon seems to be immune (Katsoyannos<br />
et al., 1998; Mavrikakis et al., 2000; Papachristos, 2007). In most areas of Greece the<br />
late autumn ripening oranges escape heavy infestation because the medfly is not active<br />
at the particular season (Katsoyannos et al., 1998; Papachristos & Papadopoulos, 2009).<br />
Today the control of the medfly is mainly carried out with the use of pesticides<br />
(Economopoulos, 1996). Mass trapping as well as the sterile insect technique have<br />
also been applied with success (Zervas, Christopoulos, & Kateva, 1997;<br />
Economopoulos et al., 1996).<br />
2.1.1. Monitoring<br />
Detection <strong>and</strong> population monitoring of C. capitata is based on trapping of adults. A<br />
wide variety of traps <strong>and</strong> trophic, optical <strong>and</strong> sexual attractants are used in trapping of<br />
the medfly, which serves for monitoring of population or for pest control.<br />
Jackson traps baited with the male specific parapheromone trimedlure are<br />
specialized for capturing males of C. capitata but these traps have low accuracy in<br />
low population densities (Katsoyannos et al., 1998). The International Pheromone<br />
Plastic McPhail trap (IPMT), baited with a water solution of a protein hydrolysate<br />
(9%) <strong>and</strong> borax (3%) added as a preservative, is the most common method for<br />
capturing female <strong>and</strong> male adults (Katsoyannos, 1994). Another trapping method<br />
using the IPMTs <strong>and</strong> the food attractants ammonium acetate (AA), 1,4<br />
diaminobutane (putrescine) <strong>and</strong> trimethylamine (TMA) (Katsoyannos,<br />
Papadopoulos, Hearth, Hendrichs, & Kouloussis, 1999a, 1999b) have been proved<br />
effective even at low <strong>and</strong> medium population levels of the medfly. In recent
IPM OF CITRUS PESTS IN GREECE<br />
33<br />
experiments it was shown that putrescine may be excluded from the traps when<br />
monitoring established populations of C. capitata (Heath, Epsky, Midgarden, &<br />
Katsoyannos, 2004).<br />
Monitoring of C. capitata <strong>by</strong> adult trapping is advised to be supported with<br />
systematic fruit collection especially <strong>by</strong> the most suceptible citrus species. Fruit<br />
sampling is considered to be an efficient warning system for early detection of the<br />
fly (Katsoyannos et al., 1998).<br />
2.1.2. Mass Trapping<br />
The method of mass trapping has been applied successfully in orange orchards<br />
(Zervas et al., 1997). Traps of reversed cup type (Zervas, 1994) baited with<br />
parapheromone trimedlure were used to attract males <strong>and</strong> the modified McPhail<br />
trap IPMT, baited with 9% food lure (hydrolyzed protein, Dacus bait) in water<br />
with the addition of 3% borax were used to attract females. Attracted medflies<br />
were killed <strong>by</strong> the insecticide methomyl. Male capturing traps were placed on<br />
orange trees at the first fortnight of September (one trap every second tree)<br />
whereas the female capturing traps were placed on orange trees 10 days later (one<br />
trap every third tree).<br />
Aiming at the reduction of cost at the use of traps in mass trapping, Zervas<br />
(1994) developed three types of low cost <strong>and</strong> easy to h<strong>and</strong>le medfly traps using a<br />
local market material. Efficacy of the new traps was similar to the commonly used<br />
traps. Two types of these traps were based on the utilisation of reversed plastic<br />
cups with trimedlure on cotton rolls as a male attractant <strong>and</strong> sugar mixted with the<br />
insecticide methomyl as a killing agent. In the third type a transparent bottle was<br />
used with a food lure (9% water solution of protein hydrolysate <strong>and</strong> 2% borax).<br />
Due to the easy manufacture <strong>and</strong> low cost, the last trap type is used with various<br />
modifications (i.e. in a lot of cases the fertilizer sulfur ammonium is placed instead<br />
of protein hydrolysate as a food attractant) <strong>by</strong> a lot of farmers for the mass trapping<br />
of medfly.<br />
Moreover, a variety of traps (yellow plastic spheres, flat yellow plates of plastic<br />
or wood, delta, glass McPhail, plastic McPhail, paper folded traps, paper envelope<br />
etc) combining visual, food <strong>and</strong> sexual stimuli have been evaluated in commercial<br />
citrus orchards with promising results (Michelakis, 1988; Liaropoulos et al., 2003;<br />
Katsoyannos & Papadopoulos, 2004).<br />
2.1.3. Biological Control<br />
Despite the long history of medfly in Greece, not enough data exist regarding the<br />
presence of native parasitoids or the establishment of exotic parasitoids that have<br />
been introduced in commercial citrus orchards for biological control. Older efforts<br />
for introduction <strong>and</strong> release of parasitoids were unsuccessful. Specifically,<br />
Dirhinus giffardii Silvestri (Hymenoptera: Chalcididae) was introduced but was<br />
not recovered (Argyriou, 1969). Test release of Opius concolor Szepligeti<br />
(Hymenoptera: Braconidae) on citrus showed that the parasitoid did not parasitize
34<br />
F. KARAMAOUNA ET AL.<br />
medfly in the field although it developed on medfly under laboratory conditions<br />
(Argyriou, 1969).<br />
Recently the presence of the parasitoid Aganaspis (Trybliographa) daci (Weld)<br />
(Hymenoptera: Eucoilidae) was recorded on infested figs on the isl<strong>and</strong> of Chios<br />
(Papadopoulos & Katsoyannos, 2003, 2007). The parasitoid exhibits high<br />
parasitism levels on medfly pupae in the field. Until today it is not known whether<br />
A. daci parasitizes C. capitata larvae in plant hosts other than figs or whether it is<br />
established in other areas of Greece. No parasitoids were found in samplings of<br />
medfly pupae in sweet oranges in Chios (Papadopoulos & Katsoyannos, 2007).<br />
Nevertheless, parasitism of C. capitata <strong>by</strong> A. daci can be an important factor for<br />
medfly control in citrus orchards in Greece as figs are one of the most important<br />
hosts contributing to the built up of C. capitata populations in late summer <strong>and</strong><br />
early autumn (Katsoyannos et al., 1998; Papadopoulos, Katsoyannos, Carey, &<br />
Kouloussis, 2001).<br />
2.1.4. Cultural Practices<br />
The succession of host fruits <strong>and</strong> their availability throughout the year is of high<br />
importance in determining overall population levels of the med fly. Thus collecting<br />
<strong>and</strong> destroying infested fruits fallen on the ground is advised as a control strategy<br />
(Katsoyannos, 1996a). In citrus orchards, the presence of bitter orange <strong>and</strong> fig<br />
trees, which are found scattered inside or at the periphery of the orchards, seem to<br />
have an important role in C. capitata population dynamics (Katsoyannos, 1983;<br />
Katsoyannos et al., 1998; Papachristos, 2007). Early in the season (May to<br />
August), the rate of population built-up depends on the availability of mature bitter<br />
oranges whereas later in the season on the presence of figs. In addition, bitter<br />
oranges <strong>and</strong> figs are highly attractive for C. capitata <strong>and</strong> seem to keep females<br />
from attacking near<strong>by</strong> hosts <strong>and</strong> dispersal (Katsoyannos, 1983; Katsoyannos et al.,<br />
1998). Elimination of these fruits or their utilization as traps on the trees can<br />
contribute in an integrated management programme of C. capitata.<br />
2.1.5. Biotechnical Methods<br />
The sterile insect technique (SIT) is considered as an environmental friendly <strong>and</strong><br />
effective control method for Tephritids fruit flies. An attempt to control C. capitata<br />
with SIT was performed in the valley of Fodele – Crete with encouraging results<br />
(Economopoulos et al., 1996; Papadopoulos & Economopoulos, 1997b).<br />
2.1.6. Chemical Control<br />
Cover <strong>and</strong> bait sprayings are the main control methods of medfly in Greece<br />
(Economopoulos, 1996). The sprays may be applied empirically based on the time<br />
of the year (Liaropoulos et al., 2003) or on systematic observations <strong>and</strong> monitoring<br />
of insect populations. Usually the bait sprays are applied from the ground using<br />
conventional sprayers <strong>and</strong> cover part of each tree or part of each two or three trees.
IPM OF CITRUS PESTS IN GREECE<br />
35<br />
A food attractant, mainly a compound that releases ammonia, is added in the<br />
pesticide solution.<br />
The timing of spray applications is determined <strong>by</strong> monitoring medfly population<br />
with traps, which are hanged on citrus trees a few weeks before fruits begin to<br />
mature. The monitoring of adult population may take place at field or region scale.<br />
Trap networks for monitoring C. capitata population have been installed <strong>and</strong><br />
operate in some areas of Greece <strong>by</strong> the Regional Plant Protection Services so<br />
forecasting of infestation is possible based on trap captures <strong>and</strong> environmental<br />
conditions <strong>and</strong> warnings are released to the growers when necessary. Although<br />
treatment application thresholds against medfly have not been established at<br />
national level, those suggested <strong>by</strong> Katsoyannos (1996a) are applied in many cases<br />
(20 adults/trap/week in autumn on clementines approaching ripeness, 40–50<br />
adults/trap/week in autumn on oranges (pre-ripe <strong>and</strong> ripe stages), 10<br />
adults/trap/week in spring on late ripening varieties).<br />
When no monitoring is performed, sprayings are performed when the fruits reach<br />
maturity whereas the number of applications depends on the region, the season <strong>and</strong><br />
the variety of citrus fruits. A spray program for orange <strong>and</strong> m<strong>and</strong>arin, which was<br />
recommended <strong>by</strong> the Ministry of Rural Development <strong>and</strong> Food in the past <strong>and</strong> can<br />
be applied even today, if using other insecticides, involves the following actions:<br />
(a) For bait spraying, the first application is carried out 15 days before fruit<br />
ripening <strong>and</strong> is repeated at 5–7 days intervals. The spray solution consists of 2%<br />
protein (as an attractant) <strong>and</strong> 0.3% dimethoate or fenthion or 0.5% malathion. It is<br />
applied on hedges <strong>and</strong> bushes in the perimeter of the orchard, on the interior <strong>and</strong><br />
the upper part of the trees, mainly on branches that do not bare fruits (b) For cover<br />
spaying, the first application is carried out at the beginning of ripening <strong>and</strong> spraying<br />
may be repeated after 20 days depending on the prevailing enviromental conditions<br />
<strong>and</strong> the time of fruit harvest. The spray solution consists of 0.03% dimethoate or<br />
fenthion or other <strong>org</strong>anophosphorate insecticides (Anonymous, 1973).<br />
In most of the orange cultivated areas in Greece the bait sprayings applied for the<br />
control of Bactrocera oleae (Gmelin) also contribute to a significant reduction of<br />
the medfly populations (Economopoulos, 1996). The same attractants (salt of<br />
protein hydrolysates) as those for the medfly have been used in bait sprays for B.<br />
oleae together with <strong>org</strong>anophophorate insecticides. Applications start early in the<br />
summer <strong>and</strong> they are continued until the end of autumn (Broumas, 1994).<br />
In some cases, spray solutions are applied on an artificial medium such as a<br />
gunny placed on a parallelepiped plastic plate which is hanged on trees branches<br />
(Economopoulos, 1996). Laboratory experiments <strong>by</strong> Mavrikakis, Remboulakis,<br />
<strong>and</strong> Economopoulos, (2003) showed that a type of a paper surface (Vioryl) baited<br />
with a water solution of protein hydrolysate (6%) had a better “attract <strong>and</strong> kill”<br />
performance on medfly than the gunny surface baited with the same food lure. The<br />
insecticide (active ingredient) used as a killing agent was spinosad in a proportion<br />
of 0.04% v/v <strong>and</strong> it was effective for a time period more than 5 weeks.<br />
Some of the former mentioned insecticidal active substances used for the control of<br />
medfly have been withdrawn after being re-evaluated (Directive 91/414/EEC) in<br />
the E.C. (fenthion, malathion). Currently, the insecticides which are authorized<br />
for use against medfly in Greece include Beauveria bassiana (m<strong>and</strong>arin),
36<br />
F. KARAMAOUNA ET AL.<br />
cypermethrin (lemon, grapefruit, m<strong>and</strong>arin, orange), flucythrinate (lemon,<br />
grapefruit, m<strong>and</strong>arin, orange) <strong>and</strong> phosmet (lemon, grapefruit, m<strong>and</strong>arin, orange)<br />
(Authorized Plant Protection Products Data Base of the Hellenic Ministry of Rural<br />
Development <strong>and</strong> Food, 2008).<br />
2.1.7. Recommended IPM Strategies<br />
In small size citrus groves, integration of cultural <strong>and</strong> chemical control of medfly is<br />
recommended whereas the biological, chemical <strong>and</strong> SIT methods may be<br />
integrated at citrus-growing areas in large scale. Collection <strong>and</strong> destroying of<br />
infested fruits fallen to the ground, fruits remaining on trees after harvest as well as<br />
fruits without commercial value (such as bitter oranges) are cultural practices of<br />
significant value in order to prevent medfly built-up population. Early population<br />
detection is crucial for a successful control thus monitoring with IPMT traps baited<br />
with AA <strong>and</strong> TMA supported <strong>by</strong> systematic fruit inspection especially of the most<br />
preferred host (bitter oranges) are required. Bait sprayings should be preferred to<br />
cover sprayings. The timing of bait spray application should be based on medfly<br />
monitoring <strong>and</strong> on treatment application threshold. As the available treatment<br />
application threshold is practically empirical there is still a dem<strong>and</strong>ing need for its<br />
accurate determination.<br />
2.2. Scale Insects<br />
Scale insects have always been on the top of the list of the economically important<br />
insect pests in citrus in Greece. Half of the most common insect pests in the Greek<br />
citrus orchards belong to the superfamily Coccoidea with the California red scale<br />
Aonidiella aurantii <strong>and</strong> the citrus mealybug Planococcus citri being the most<br />
frequently found ones among all. In addition, a number of less important species<br />
are known to cause local outbreaks. In the past, the Mediterranean black scale<br />
Saissetia oleae was considered to be a major pest but after the introduction <strong>and</strong><br />
successful establishment of several exotic parasitoids, its population is kept below<br />
the economic injury level. At present, the Chinese wax scale Ceroplastes<br />
floridensis <strong>and</strong> the cottony-cushion scale Icerya purchasi can cause local outbreaks<br />
in specific regions in Peloponnese (Stathas, personal communication) whereas high<br />
populations of Ceroplastes rusci, Lepidosaphes beckii <strong>and</strong> Saissetia oleae are<br />
occasionally recorded too (Hellenic Ministry of Rural Development <strong>and</strong> Food,<br />
2007, unpublished data).<br />
Although considerable effort has been imposed to develop sustainable control<br />
methods of scale insects based on the use of biological control agents <strong>and</strong> the<br />
minimization of the use of chemical pesticides, spraying with insecticides is still<br />
used for the control of scale insects in citrus. Currently the most common practice<br />
in control of main scales of citrus is spray applications following the forecasts <strong>and</strong><br />
instructions issued <strong>by</strong> the Regional Plant Protection Services, which are based on<br />
population monitoring with traps <strong>and</strong>/or visual observations.
IPM OF CITRUS PESTS IN GREECE<br />
37<br />
2.2.1. Sampling <strong>and</strong> Monitoring<br />
An efficacious monitoring system is prerequisite for having a successful<br />
forecasting/warning system for citrus scale insects. A number of monitoring tools<br />
are available for citrus scales, which are used in Greece. Sex pheromone traps are<br />
utilized for the detection, monitoring <strong>and</strong> forecasting outbreaks of the California<br />
red scale A. aurantii. White sticky sex-pheromone baited traps are used for<br />
monitoring purposes of other armoured scales. Pheromone traps are also available<br />
for the citrus mealybug P. citri. Field observations <strong>and</strong> sampling are necessary for<br />
the detection of other citrus scales. Various detailed sampling schemes have been<br />
proposed for this area of concern (Katsoyannos, 1996a).<br />
2.2.2. Biological Control<br />
An extended trial has been directed toward classical biological control of citrus<br />
scales in the past so Greece is a good example of a country where native scale<br />
insects have been controlled <strong>by</strong> exotic natural enemies, both parasitoids <strong>and</strong><br />
predators. Eleven parasitoid species have been introduced, seven of them providing<br />
sufficient control whereas several predators associated with classical biological<br />
control of scale insects are frequently present in the Greek citrus orchards.<br />
Five parasitoid species, Aphytis melinus DeBach, A. lingnanensis Compere,<br />
A. coheni De Bach Compere (Hymenoptera: Aphelinidae), Encarsia perniciosi<br />
(Tower) (Hymenoptera: Aphelinidae) <strong>and</strong> Comperiella bifasciata Howard<br />
(Hymenoptera: Encyrtidae) were introduced <strong>and</strong> released in field trials against<br />
A. aurantii between 1962 <strong>and</strong> 1970. A. melinus is the leading parasitoid targeting<br />
the California red scale but its efficacy is reduced in cases of outbreaks.<br />
Comperiella bifasciata had a minor establishment whereas A. lingnanensis <strong>and</strong> A.<br />
coheni failed to be established (Katsoyannos, 1996a).<br />
Aphytis lepidosaphes Compere <strong>and</strong> Aphytis melinus DeBach were established<br />
after introduction in 1962 <strong>and</strong> they sufficiently controlled L. beckii <strong>and</strong><br />
Chrysomphalus dictyospermi M<strong>org</strong>an (Hemiptera: Diaspididae) respectively,<br />
which were major pests of citrus in the past (Katsoyannos, 1996a).<br />
The parasitoid Leptomastix dactylopii Howard (Hymenoptera: Encyrtidae) was<br />
released in Crete twice (in 1975 <strong>and</strong> 1981) for the control of the citrus mealybug<br />
P. citri but failed to get established (Katsoyannos, 1996a). Moreover, three<br />
coccinellid predators were introduced, Nephus reunioni (1977), Nephus sidi (1992)<br />
<strong>and</strong> Cryptolaemus montrouzieri Mulsant (several attempts: 1933, 1964, 1965,<br />
1969, 1977). Establishment of the Nephus spp. was not reported, however, C.<br />
montrouzieri Mulsant, which was the most effective of the three species, could not<br />
overwinter in most regions (Katsoyannos, 1996a).<br />
Four parasitoid species, Metaphycus helvolus Compere, M. bartletti Annecke &<br />
Mynhardt, M. swirskii Annecke & Mynhardt (Hymenoptera: Encyrtidae) <strong>and</strong><br />
Diversinervus elegans Silvestri (Hymenoptera: Encyrtidae) targeted the control of<br />
Saissetia oleae with relatively sufficient results (Argyriou, 1986). The coccinellid<br />
predator Rhyzobius forestieri (Mulsant) was released 25 years ago on the isl<strong>and</strong> of<br />
Chios <strong>and</strong> it is now the most abundant coccinellid found in citrus orchards. The
38<br />
F. KARAMAOUNA ET AL.<br />
predator preys mainly on soft scales, such as S. oleae <strong>and</strong> Coccus<br />
pseudomagnoliarum (Kuwana) (Hemiptera: Coccidae), which maintain at<br />
acceptable levels (Katsoyannos, 1997).<br />
Populations of the cottony-cushion scale Icerya purchasi Kaussari (Hemiptera:<br />
Margarodidae) were regulated <strong>by</strong> the introduced coccinellid predator Rhodolia<br />
cardinalis Mulsant (Katsoyannos, 1996a). Localized outbreaks of the pest have<br />
been occurring until recently but nowadays the predator is available to the growers<br />
for augmentative releases.<br />
Besides the classical biological control, naturally occurring biological control is<br />
a widespread phenomenon in Greek citrus orchards. Many indigenous parasitoids<br />
<strong>and</strong> predators are found to parasitize <strong>and</strong> prey on citrus scale insects. Three<br />
indigenous parasitoids [Aphytis chrysomphali (Mercet), Aphytis chilensis Howard<br />
<strong>and</strong> Encarsia citrina (Craw)] <strong>and</strong> three predators [the coccinellids Rhyzobius<br />
lophanthae (Blaisdell) <strong>and</strong> Chilocolus bipustulatus (L.) <strong>and</strong> the nitidulid<br />
Cybocephalus fodori (Endrodi-Younga)] are the most common species that<br />
contribute to the suppression of the armoured scales in citrus, with the predator R.<br />
lophanthae being the most important one (Katsoyannos, 1996a).<br />
A considerable number of indigenous natural enemies are related to the control<br />
of the citrus mealybug; the parasitoids Anagyrus pseudococci (Girault) <strong>and</strong><br />
Leptomastidea abnormis (Girault) (both Hymenoptera: Encyrtidae) along with the<br />
predators Nephus includens (Kirsch) <strong>and</strong> N. bisignatus (Boheman) (Coleoptera:<br />
Coccinellidae) contribute substantially to its control (Katsoyannos, 1996a;<br />
Kontodimas, Eliopoulos, Stathas, & Economou, 2004). Among the various<br />
parasitoid species associated with soft scales in citrus, Tetrastichus ceroplastae<br />
(Girault) (Hymenoptera: Eulophidae) <strong>and</strong> Scutellista cyanea Motschulsky<br />
(Hymenoptera: Pteromalidae) are the most frequent species that parasitize<br />
Ceroplastes rusci <strong>and</strong> C. floridensis Comstock (Katsoyannos, 1996a; Stathas,<br />
Kavallieratos, & Eliopoulos, 2003).<br />
In general citrus-infesting scale insects are adequately retained at low levels <strong>by</strong><br />
the activity of introduced <strong>and</strong>/or native parasitoids <strong>and</strong> predators. However, in<br />
cases where locally outbreaks occur due to various factors, further action is needed<br />
to suppress the infestation below the economic injury level. Augmentative releases<br />
of natural enemies were performed in the past against the citrus mealybug P. citri<br />
<strong>and</strong> the soft scales S. oleae <strong>and</strong> C. pseudomagnoliarum using the coccinellid<br />
predators Cryptolaemus montrouzieri <strong>and</strong> Exochomus quadripustulatus (L.)<br />
respectively (Katsoyannos, 1996a). Presently augmentative releases are performed<br />
sporadically against P. citri using the coccinellid predators Nephus includens <strong>and</strong><br />
N. bisignatus with very satisfying results, especially in <strong>org</strong>anic citrus orchards. Growers<br />
occasionally use Rhodolia cardinalis to suppress local outbreaks of I. purchasi; the<br />
predator has been commercially available in the Greek market since 2006.<br />
2.2.3. Cultural Practices<br />
Cultural techniques involve a series of modifications of the st<strong>and</strong>ard management<br />
practices in order to prevent or make the environment less favorable for the
IPM OF CITRUS PESTS IN GREECE<br />
39<br />
reproduction, dispersal <strong>and</strong>/or survival of scale insects. Reduced fertilizers input<br />
<strong>and</strong> irrigation regimes are conidered to moderate the susceptibility of the trees to<br />
scale insects infestation. Since scale insects are favored <strong>by</strong> low light <strong>and</strong> high<br />
humidity conditions, which are favoured <strong>by</strong> dense foliage, pruning of trees in<br />
spring should be regulated to enhance air movement <strong>and</strong> sunlight infusion into the<br />
canopy <strong>and</strong> hence to minimize survival <strong>and</strong> establishment of high populations of<br />
the pests in the orchards (Katsoyannos, 1996a).<br />
2.2.4. Chemical Control<br />
Chemical control of citrus scale insects following monitoring of the population<br />
with traps <strong>and</strong> visual observations is a common practice in Greece. Insecticides<br />
(active substances) authorized for use against the California red scale <strong>and</strong> the citrus<br />
mealybug in Greece include buprofezin (citron, lemon, grapefruit, m<strong>and</strong>arin,<br />
orange; only A. aurantii: bitter orange), chlorpyrifos (lemon, grapefruit, m<strong>and</strong>arin,<br />
orange, pumelo), cypermethrin (lemon, grapefruit, m<strong>and</strong>arin, orange), flucythrinate<br />
(lemon, grapefruit, m<strong>and</strong>arin, orange), paraffin oil (lemon, grapefruit, m<strong>and</strong>arin,<br />
orange, pumelo; only A. aurantii: bitter orange), petroleum oil (lemon, grapefruit,<br />
m<strong>and</strong>arin, orange), phosmet (lemon, grapefruit, m<strong>and</strong>arin, orange), pyriproxyfen<br />
(only A. aurantii: lemon, m<strong>and</strong>arin, orange) <strong>and</strong> white oil (lemon, grapefruit,<br />
m<strong>and</strong>arin, orange). Some of these active substances are registered for the control of<br />
other armoured scales <strong>and</strong> soft scales in citrus whereas chlorpyrifos-methyl <strong>and</strong><br />
fenoxycarb are added in the pesticide list against Aspidiotus nerii (only<br />
chlorpyrifos methyl) <strong>and</strong> Saissetia oleae (Authorized Plant Protection Products<br />
Data Base of the Hellenic Ministry of Rural Development <strong>and</strong> Food, 2008).<br />
2.2.5. Recommended IPM Strategies<br />
A good monitoring system that provides the necessary information for early scale<br />
detection <strong>and</strong> the status of natural enemies is essential for the selection of the<br />
sufficient control measures. In general, natural enemies provide adequate control of<br />
the citrus-infesting scales except in cases that outbreaks A. aurantii occur; the lack<br />
of an efficient predator against the California red scale makes it difficult to<br />
suppress the pest at high population levels. Therefore, conservation of existing<br />
natural enemies <strong>and</strong> augmentative releases of insectary-reared parasitoids <strong>and</strong><br />
predators are very important in maintaining the scales population at low levels.<br />
Accessory cultural techiques (i.e. pruning in spring <strong>and</strong> moderate use of fertilizers<br />
<strong>and</strong> irrigation in summer) contribute in keeping the scale numbers low. In cases<br />
insecticide application is required (e.g. when widespread increase of the California<br />
red scale populations or the citrus mealybug outbreaks occur) one or two welltimed<br />
cover sprays may be applied <strong>by</strong> using selective insecticides. Less selective<br />
chemicals should be applied only spotted or in extreme situations on heavily<br />
infested areas of the grove (aiming also at the protection <strong>and</strong> conservation of<br />
natural enemies).
40<br />
F. KARAMAOUNA ET AL.<br />
2.3. Whiteflies<br />
Three exotic whitefly species have invaded Greece during the last three decades,<br />
the citrus whitefly Dialeurodes citri in 1973 (Pappas & Viggiani, 1979; Pappas,<br />
1981), the Japanese bayberry whitefly Parabemisia myricae (Kuwana) (Hemiptera:<br />
Aleyrodidae) in 1989 (Michalopoulos, 1989; Michelakis & Alex<strong>and</strong>rakis, 1989)<br />
<strong>and</strong> the woolly whitefly Aleurothrixus floccosus in 1991 (Katsoyannos, 1991),<br />
which caused considerable economic yield losses in citrus orchards especially in<br />
the early years after the invasion. Among the three species the woolly whitefly<br />
caused the most serious problems to the citrus growers. Woolly <strong>and</strong> citrus<br />
whiteflies are still considered to be main insect pests locally (Kalaitzaki,<br />
Alex<strong>and</strong>rakis, Varikou, & Pervolarakis, 2003; Kontodimas et al., 2005). However,<br />
all three species are excellent examples of efficient biological control in practice.<br />
2.3.1. Sampling <strong>and</strong> Monitoring<br />
The Japanese bayberry whitefly prefers to oviposit on incompletely exp<strong>and</strong>ed new<br />
leaves whereas woolly <strong>and</strong> citrus whiteflies prefer completely exp<strong>and</strong>ed but not yet<br />
dark green young leaves. In any case, sampling of infested young leaves <strong>and</strong> their<br />
examination under a stereoscopic microscope is necessary in order to assess the<br />
infestation level <strong>and</strong> the efficiency of any natural enemies (mainly the rate of<br />
parasitism). At the same time visual observation should be done in order to record<br />
the relative infestation intensity of the citrus trees. In addition, yellow sticky traps<br />
could considerably help to record the first flights of the whiteflies’ adults as well as<br />
to monitor the annual fluctuation of the population of whiteflies <strong>and</strong> their natural<br />
enemies.<br />
2.3.2. Biological Control <strong>and</strong> Cultural Practices<br />
All the whitefly species were exotic, hence their biological control was based on<br />
the introduction of their natural enemies, especially parasitoids (classical biological<br />
control).<br />
The control of Dialeurodes citri was achieved <strong>by</strong> the introduction of the<br />
parasitoid Encarsia lahorensis (Howard) (Hymenoptera: Aphelinidae) on the<br />
isl<strong>and</strong> of Corfu in 1976 (Pappas & Viggiani, 1979). By 1994, the parasitoid was<br />
well established <strong>and</strong> was found in almost all citrus orchards in the mainl<strong>and</strong><br />
(Katsoyannos, 1996a); it was also imported <strong>and</strong> released on the isl<strong>and</strong> of Crete in<br />
2003 (Kalaitzaki et al., 2003).<br />
Control of Parabemisia myricae was attempted with the parasitoid Eretmocerus<br />
deBachi Rose <strong>and</strong> Rosen (Hymenoptera: Aphelinidae), which was introduced <strong>and</strong><br />
released in Crete in 1990 <strong>and</strong> 1991, but no data regarding its establishment are<br />
available (Katsoyannos, 1996a). However, the presence of P. myricae is rare after<br />
the introduction of E. deBachi.<br />
In case of Aleurothrixus floccosus, the parasitoid Cales noacki Howard<br />
(Hymenoptera: Aphelinidae) was introduced in 1991 <strong>and</strong> augmentation of its<br />
population in the insectary followed. During the years 1992–1995 more than 30
IPM OF CITRUS PESTS IN GREECE<br />
41<br />
million individuals of the parasitoid were released in more than 300 sites of citrusgrowing<br />
areas of the country. In most of these areas the control of the woolly<br />
whitefly was achieved during 1995 (infestation level 1 nymph/cm 2 ) of A. floccosus is<br />
recommended (Katsoyannos et al., 1998).<br />
Rearing of C. noacki in insectaries is suggested for augmentative biological<br />
control of A. floccosus, which in addition could serve as a useful deposit in case of<br />
invasion of the quarantine pest citrus blackfly Aleurocanthus woglumi Ash<strong>by</strong><br />
(Hemiptera: Aleyrodidae) (A1 EPPO List).
42<br />
F. KARAMAOUNA ET AL.<br />
2.4. The Citrus Leafminer, Phyllocnistis citrella<br />
The citrus leafminer Phyllocnistis citrella was first recorded in Greece on the isl<strong>and</strong><br />
of Rhodes (southeastern Greece) <strong>and</strong> in Crete in June 1995 (Anagnou-Vernoniki,<br />
1995; Michelakis & Vacante, 1997). More recordings of the pest followed on other<br />
Greek isl<strong>and</strong>s (Cos, Astipalea, Lesvos, Chios, Samos <strong>and</strong> Paros) <strong>and</strong> in the<br />
mainl<strong>and</strong> (Attica <strong>and</strong> Laconia-Peloponnese) in July <strong>and</strong> August, 1995 (Anagnou-<br />
Vernoniki, 1995). After a few months the citrus leafminer was found in almost all<br />
citrus growing areas of Greece (Tsagarakis, Kalaitzaki, Lykouressis, Michelakis, &<br />
Alex<strong>and</strong>rakis, 1999).<br />
Upon introduction of the pest, quarantine <strong>and</strong> other regulatory measures were<br />
enforced but they had a very limited impact on the spread of the pest which very<br />
rapidly invaded all citrus cultivated areas in the state. The growers were advised<br />
not to overuse <strong>and</strong>/or misuse insecticides as experience from other countries had<br />
shown that the chemical control was a short term <strong>and</strong> expensive solution due to the<br />
long vegetative period of citrus <strong>and</strong> the large number of generations of citrus<br />
leafminer per year. Furthermore, chemicals would have unfavorable side effects on<br />
the existing effective biological control of other citrus pests <strong>and</strong> there was a<br />
possibility of resistance development of the citrus leafminer to insecticides.<br />
Nevertheless, many growers tried to apply insecticides but soon they had to<br />
admit that chemicals were an inadequate solution to the problem. Moreover,<br />
chemical control using broad spectrum insecticides was indeed putting at risk the<br />
Integrated Pest Management of citrus insect pests, such as scales <strong>and</strong> aphids as<br />
well as the successful biological control of the woolly whitefly Aleurothrixus<br />
floccosus <strong>by</strong> disruption of the newly established exotic parasitoid Cales noacki.<br />
Biological control, on the other h<strong>and</strong>, was known to be the most effective method<br />
of managing the citrus leafminer in commercial orchards (Hoy et al., 1995; Neale,<br />
Smith, Beattie, & Miles, 1995; Smith & Beattie, 1996; Argov & Rössler, 1996).<br />
Therefore the impact of the native natural enemies was studied <strong>and</strong> classical<br />
biological control <strong>by</strong> introduction <strong>and</strong> release of the most promising parasitoid<br />
species in two sites (Crete <strong>and</strong> Peloponnese) was attempted (Kalaitzaki, 2004). In<br />
addition cultural measures to prevent dispersal were strongly recommended <strong>by</strong> the<br />
agronomists/consultants to the citrus growers (Michelakis & Vacante, 1997).<br />
Early studies after the implementation of the classical biological control<br />
programme of the citrus leafminer in Crete showed that the number of immature<br />
individuals of the citrus leafminer/leaf fluctuated from 0.1–3.9 to 0.01–1.06 on<br />
orange trees <strong>and</strong> m<strong>and</strong>arin trees, respectively (with m<strong>and</strong>arin being more resistant to<br />
infestation) (Kalaitzaki, 2004). Five peaks of the live immature individuals of the<br />
citrus leafminer/leaf were recorded on orange trees (two in summer: end of May <strong>and</strong><br />
mid June <strong>and</strong> three in autumn: end of September, end of October <strong>and</strong> mid November)<br />
<strong>and</strong> four peaks on m<strong>and</strong>arin trees (mid June, end of September, end of October,<br />
beginning of December) (Kalaitzaki, 2004). Lower levels of infestation (0.017–1.76<br />
live immature individuals/per leaf) were recorded in Argolis-Peloponnese, the second<br />
area of the parasitoids’ release (Tsagarakis et al., 1999). Later studies (2004 <strong>and</strong><br />
2005) on the isl<strong>and</strong>s of Lesvos <strong>and</strong> Chios <strong>and</strong> in western mainl<strong>and</strong> revealed low<br />
infestation of the citrus leafminer i.e. 0.06–0.58, 0.08–0.72 <strong>and</strong> 0.04–0.82 immature
IPM OF CITRUS PESTS IN GREECE<br />
43<br />
individuals/leaf respectively. As a final point the citrus leafminer causes problems<br />
particularly on young citrus trees <strong>and</strong> overgraftings in nurseries but its damage on<br />
adult trees under Mediterranean conditions lacks economic importance (Garcia-Marí,<br />
Gr<strong>and</strong>a, Zaragoza, & Agusti, 2002).<br />
2.4.1. Sampling <strong>and</strong> Monitoring<br />
Sampling for monitoring infestation <strong>by</strong> the citrus leafminer involves collection of<br />
new shoots <strong>and</strong> leaves from growth flushes <strong>and</strong> observation of mines. The<br />
economic threshold for a chemical application on citrus leafminer has been<br />
estimated <strong>by</strong> several researchers; in China it is 0.74 larvae/leaf (or percentage of<br />
leaf damage over 20%) (Huang & Li, 1989); in Australia it is fixed at 25% of<br />
shoots with leaves smaller than 3 cm exhibiting mines of L1 (Beattie & Smith,<br />
1993); in Florida it is set at 30% of young shoots baring mines with live larvae<br />
(sampling should be performed when half of the trees in the orchard have young<br />
shoots) (Knapp et al., 1995).<br />
2.4.2. Biological Control<br />
Five exotic hymenopteran parasitoid species were introduced from Cyprus in 1996<br />
<strong>and</strong> were subsequently mass reared in the insectary of the Institute of Subtropical<br />
Crops <strong>and</strong> Olive (National Agricultural Research Foundation) in Chania-Crete. The<br />
introduced species were the encyrtid Ageniaspis citricola Logvinovskaya<br />
(Hymenoptera: Encyrtidae) <strong>and</strong> the eulophids Cirrospilus quadristriatus (Subba<br />
Rao <strong>and</strong> Ramamani), Citrostichus phyllocnistoides (Narayanan), Quadrastichus sp.<br />
<strong>and</strong> Semielacher petiolatus (Girault) (Hymenoptera: Eulophidae). A small number<br />
of all parasitoids were released in 1996 but cultures of Ageniaspis citricola <strong>and</strong><br />
Cirrospilus quadristriatus could not be kept after the first year <strong>and</strong> hence these<br />
species did not establish (Kalaitzaki, 2004).<br />
Citrostichus phyllocnistoides, Quadrastichus sp. <strong>and</strong> Semielacher petiolatus were<br />
released systematically (100–250 individuals/species/10 days from June to November)<br />
in orange <strong>and</strong> m<strong>and</strong>arin orchards in Crete (Chania) <strong>and</strong> the impact of both native <strong>and</strong><br />
introduced parasitoids was studied from 1997 to 1999. Similar releases were also<br />
performed in Peloponnese (Argolis, Korinthia, Lakonia) (Tsagarakis et al., 1999).<br />
All of the released parasitoid species established in Crete <strong>and</strong> contributed to the<br />
reduction of the citrus leafminer population, especially Citrostichus<br />
phyllocnistoides which dispersed very rapidely <strong>and</strong> far from the release sites <strong>and</strong> it<br />
achieved the highest percentage parasitism (mean 15.2–20.8% <strong>and</strong> maximum 45.8–<br />
51.1% on m<strong>and</strong>arin <strong>and</strong> orange trees, respectively).<br />
Only a few native parasitoid species were found to parasitize the citrus leafminer in<br />
Crete i.e. Pnigalio pectinicornis L., Neochrysocharis formosa (Westwood) <strong>and</strong><br />
Cirrospilus pictus (Nees) (all Hymenoptera: Eulophidae) in very small numbers <strong>and</strong><br />
with small contribution in percentage parasitism of the citrus leafminer (Kalaitzaki,<br />
Lykouressis, & Michelakis 1999; Kalaitzaki, 2004). Among them, P. pectinicornis was<br />
the most abundant one (Kalaitzaki et al., 1999; Kalaitzaki, Lykouressis, Perdikis, &
44<br />
F. KARAMAOUNA ET AL.<br />
Alex<strong>and</strong>rakis, 2007). Results of the second release site differ. Th e exoti c parasitoids<br />
C. phyllocnistoides <strong>and</strong> S. petiolatus were recovered whereas Quadrastichus sp. was not<br />
recovered (Tsagarakis et al., 1999). Although the population of C. phyllocnistoides<br />
increased with time after the release, the exotic parasitoid did not displace the native<br />
species N. formosa <strong>and</strong> P. pectinicornis. Neochrysocharis formosa was the most<br />
abundant parasitoid for a period of 3 years after the release (Tsagarakis & Lykouressis,<br />
2002; Tsagarakis, Kalaitzaki, Lykouressis, Michelakis, & Alex<strong>and</strong>rakis, 2003).<br />
Citrostichus phyllocnistoides has been found in almost all citrus producing areas in<br />
Greece (Kalaitzaki, 2004).<br />
The parasitoids Pnigalio sp., Cirrospilus sp., N. formosa <strong>and</strong> C. phyllocnistoides<br />
were collected at the areas of Marathonas-Attiki, Galatas-Trizinia <strong>and</strong> Skala-Lakonia in<br />
1999–2000 (Anagnou-Veroniki, Doukas, & Kontodimas, 2002), Pnigalio pectinicornis<br />
<strong>and</strong> Cirrospilus sp. were collected on the isl<strong>and</strong>s of Lesvos <strong>and</strong> Chios <strong>and</strong> in western<br />
mainl<strong>and</strong>, as were N. formosa <strong>and</strong> C. phyllocnistoides (Papanikolaou, 2005).<br />
The list of native parasitoids exp<strong>and</strong>ed with the first recording of Pnigalio soemius<br />
(Walker) (Hymenoptera: Eulophidae) (Papanikolaou, 2005; Papanikolaou,<br />
Kavallieratos, Kontodimas, & Tomanovic, 2006) <strong>and</strong> Semielacher silvicola Boucek<br />
(Hymenoptera: Eulophidae) in Attica, in 2005 (Vamvakas, Anagnou-Veroniki, &<br />
Kontodimas, 2005).<br />
2.4.3. Cultural Practices<br />
Cultural measures advised involve some changes of the st<strong>and</strong>ard management practices<br />
in order to prevent or make the environment less favorable for the pest reproduction,<br />
dispersal <strong>and</strong>/or survival. Decrease of fertilization <strong>and</strong> irrigation inputs should moderate<br />
the susceptibility of the new flush to the citrus leafminer during summer when the pest<br />
is very active. Moreover, fertilization, irrigation <strong>and</strong> pruning should be regulated to<br />
enhance discrete flush patterns over large areas, breaking generations overlap<br />
(Anagnou-Veroniki, Volakakis, & Gianoulis, 1995; Michelakis & Vacante, 1997).<br />
2.4.4. Chemical Control<br />
The application of insecticides to control the citrus leafminer is proved to be a<br />
short term solution especially for plant nurseries <strong>and</strong> newly grafted trees which<br />
suffer more from the pest infestation.<br />
The insecticides (active substances) which were initially recommended were<br />
fenoxycarb <strong>and</strong> diflubezuron in combination with summer oils. Only the external part<br />
of the trees, where the flushes <strong>and</strong> hence the citrus leafminer infestation occurs,<br />
should be sprayed with the solutions. Fenoxycarb showed no killing effects on<br />
C. noacki, the parasitoid of A. floccosus (Buchelos & Foudoulakis, 2000). Later on<br />
more selective insecticides i.e. chlorfenapyr, abamectin, flufenoxuron, azadirachtin,<br />
summer oils etc. were used (Michelakis & Vacante, 1997).<br />
Other insecticides added in the list were acephate, diazinon, dimethoate,<br />
methomyl, phospanidon, fenvalarate whereas their side effects on the natural<br />
enemies of the pest were illustrated (Anagnou-Veroniki et al., 1995).
IPM OF CITRUS PESTS IN GREECE<br />
45<br />
Today the list with the registered insecticides for use against the citrus leafminer<br />
in Greece includes acetamiprid, (in nurseries for lemon, m<strong>and</strong>arin <strong>and</strong> orange),<br />
azadirachtin (grapefruit, lemon, m<strong>and</strong>arin, orange), buprofezin (bitter orange),<br />
flufenoxuron (lemon, orange) imidacloprid (grapefruit, lemon, m<strong>and</strong>arin, orange),<br />
methoxyfenozide (m<strong>and</strong>arin, orange), paraffin oil (bitter orange), tebufenozide<br />
(m<strong>and</strong>arin) <strong>and</strong> thiamenthoxam (lemon, m<strong>and</strong>arin, orange) (Authorized Plant<br />
Protection Products Data Base of the Hellenic Ministry of Rural Development <strong>and</strong><br />
Food, 2008).<br />
2.4.5. Recommended IPM Strategies<br />
Manipulation of the timing <strong>and</strong> quantities of irrigation <strong>and</strong> fertilizers provided <strong>and</strong><br />
pruning in order to separate the main growth flushes (spring–summer–autumn) <strong>and</strong><br />
decrease the susceptibility of the summer flush, when the citrus leafminer is active,<br />
contributes to maintenance of the pest populations at low levels (Anagnou-Veroniki,<br />
1995; Katsoyannos, 1996a, 1996b; Michelakis & Vacante, 1997). Conservation of<br />
the established exotic parasitoids <strong>and</strong> native beneficials is essential for the control of<br />
the citrus leafminer in the productive orchards. Chemical treatments using selective<br />
insecticides for the control of the pest should be restricted in the nurseries.<br />
2.5. Aphids<br />
Commonly, aphids can be very important pests in citrus-growing areas under<br />
favourable environmental conditions due to their high reproductive potential which<br />
results in several generations per year <strong>and</strong> the production of alate adults which can spread<br />
very quickly <strong>and</strong> migrate to great distances (Kavallieratos et al., 2005; Athanassiou,<br />
Kavallieratos, Tomanović, Tomanović, & Milutinović, 2005). Nevertheless, aphids<br />
infesting citrus in Greece <strong>and</strong> generally in the northern Mediterranean countries are<br />
most often kept in low numbers under biological control <strong>by</strong> several indigenous<br />
parasitoids <strong>and</strong> predators (Katsoyannos, 1996a).<br />
Nine aphid species have been reported to infest citrus trees in Greece, which refer<br />
to Aphis craccivora Koch, Aphis gossypii Glover, Aphis spiraecola Patch,<br />
Aulacorthum solani (Kaltenbach), Brachycaudus helichrysi (Kaltenbach),<br />
Macrosiphum euphorbiae (Thomas), Myzus persicae (Sulzer), Rhopalosiphum<br />
maidis (Fitch) <strong>and</strong> Toxoptera aurantii (Boyer de Fonscolombe) (Kavallieratos &<br />
Lykouressis, 1999). The exotic Aphis spiraecola <strong>and</strong> the indigenous Toxoptera<br />
aurantii <strong>and</strong> Aphis gossypii are the most important aphid species on citrus in the<br />
region (Argyriou, 1969).<br />
Strict monitoring <strong>and</strong> quarantine procedures must be followed for continued<br />
exclusion from the EPPO region of Toxoptera citricida (Kirkaldy) (EPPO A2 List,<br />
2004), which is the highest potency vector for Citrus Tristeza Closterovirus (CTV)<br />
causing the homonymous destructive virus disease of citrus.<br />
Aphis gosypii is also an efficient vector of many isolates of CTV, whereas T. aurantii<br />
is a less efficient vector. The prevention of aphids’ population outbreaks is primarily<br />
based on conservation <strong>and</strong>, possibly, stimulation of the activity of their natural<br />
enemies (Katsoyannos, 1996a).
46<br />
F. KARAMAOUNA ET AL.<br />
2.5.1. Sampling <strong>and</strong> Monitoring<br />
During spring, yellow water-pan traps are used <strong>and</strong> visual inspections are carrried<br />
out for monitoring citrus aphids. Moericke pan-traps, both square (60 × 60 × 10 cm)<br />
<strong>and</strong> round (30 cm in diameter), painted canary yellow inside <strong>and</strong> containing<br />
water up to depth of 3–4 cm with a spoonful of added detergent, are commonly<br />
used. They are placed in the citrus groves in mid-spring (density 2–5 traps/ha at a<br />
height of 70 cm above the ground) <strong>and</strong> they are checked once or twice per week<br />
during the growing season. Information about citrus aphids populations provided<br />
<strong>by</strong> 12 m high suction traps, if available, might also be useful (Katsoyannos,<br />
1996a).<br />
Inspections, especially on the apical twigs of new growth flushes, are made<br />
weekly during the growing season. Curled newer leaves, honeydew, sooty mould<br />
<strong>and</strong> the presence of ants are signs aiding the detection of foci of aphid infestation<br />
in an orchard. Rates of parasitism are monitored <strong>by</strong> examination of aphids on<br />
sampled leaves <strong>and</strong> twigs.<br />
Aphidophagous coccinellid population levels are monitored using visual<br />
inspections <strong>and</strong> <strong>by</strong> heating branches of trees with a rubber-covered stick over a<br />
1 m 2 cloth screen <strong>and</strong> recording the numbers of adults <strong>and</strong> larvae of the beetles thus<br />
dislodged (Katsoyannos, 1984).<br />
2.5.2. Biological Control<br />
Control of citrus aphids is mainly based on natural enemy manipulation<br />
(conservation) in pest management. Aphids have several natural enemies which<br />
most often suppress the pests below levels of economic concern. Indigenous<br />
parasitoids which have been reported to parasitize aphids in Greece include the<br />
hymenopteran Aphidiinae parasitoids Aphidius colemani Viereck, Aphidius<br />
matricariae Haliday, Aphidius urticae Haliday, Diaeretiella rapae (M’Intosh),<br />
Ephedrus persicae Froggat, Lysiphlebus confusus Tremblay <strong>and</strong> Eady, Lysiphlebus<br />
fabarum (Marshall), Lysiphlebus testaceipes (Cresson), Praon volucre (Haliday),<br />
Binodoxys acalephae (Marshall) <strong>and</strong> Binodoxys angelicae (Haliday) (Kavallieratos &<br />
Lykouressis, 1999; Kavallieratos et al., 2001; Kavallieratos, Stathas, &<br />
Tomanović, 2002; Kavallieratos & Lykouressis, 2004).<br />
Alloxysta spp., Asaphes vulgaris Walker, Asaphes spp., Dendrocerus spp.,<br />
Pachyneuron aphidis (Bouché), Pachyneuron spp., Phaenoglyphis spp. <strong>and</strong><br />
Syrphophagus aphidivorus (Mayr) have been reported as hyperparasitoids that<br />
attack primary parasitoids of aphids infesting citrus (Santas, 1979; Kavallieratos &<br />
Lykouressis, 1999).<br />
Coccinellidae predators Coccinella septempunctata L., Adalia bipunctata L.,<br />
Propylea quatuordecimpunctata L., Hippodamia variegate (Göeze), Oenopia<br />
(Synharmonia) conglobata L., Adalia decempunctata L. <strong>and</strong> Scymus (Pullus)<br />
subvillosus (Göeze) are frequent in Greece. Other aphid predators belong to the<br />
Syrphidae such as Epistrophe baiteata (De Greer), Paragus albifrons Meigen,<br />
Paragus majaranae Rondani, Scaeva albomaculata Macquart, Syrphus<br />
latefasciatus Macquart, <strong>and</strong> Sphaerophoria sp. The green lacewing Chrysoperla
IPM OF CITRUS PESTS IN GREECE<br />
47<br />
carnea (Chrysopidae) Stephens is a notable aphid predator in Greece too<br />
(Katsoyannos, 1996a).<br />
Conservation of these agents includes management practices e.g. avoiding<br />
chemical treatment, especially between mid-spring <strong>and</strong> early summer. Long-term<br />
positive effects on the naturally-occurring biological control of citrus aphids are<br />
obtained <strong>by</strong> preserving existing habitats, which function as reservoirs of the natural<br />
enemies, or <strong>by</strong> creating new ones where needed.<br />
In general, preserving sufficient plant diversity in the agroecosystem is<br />
desirable, since it ensures the continuous presence of other aphid species which<br />
serve as alternative prey of coccinellids during the summer scarcity of citrus<br />
aphids. Other important measures include preserving hibernation sites <strong>and</strong><br />
preventing ants (Formicidae) from tending aphid colonies <strong>and</strong> disturbing the<br />
aphids’ natural enemies. Although, these methods are indirect <strong>and</strong> their effect is<br />
difficult to be evaluated, they are cost effective <strong>and</strong> easy to implement<br />
(Katsoyannos, 1996a).<br />
A classical biological control case involved the release of the predator<br />
Harmonia axyridis Pallas (Coleoptera: Coccinellidae) in citrus in experimental<br />
fields in Marathon (Attica), on Chios isl<strong>and</strong>, in Leonidion (Peloponnese) <strong>and</strong> in<br />
Chania (Crete) in 1994. The predator was highly efficient against aphid population<br />
outbreaks (Katsoyannos, Kontodimas, Stathas, & Tsartsalis, 1995). However, when<br />
sampling was contacted between 1995 <strong>and</strong> 1999 there was no evidence for the<br />
establishment of H. axyridis in the release sites (Kontodimas et al., 2008). Only<br />
small colonies of overwintered adults (
48<br />
F. KARAMAOUNA ET AL.<br />
cultural practices. Conservation of aphidophagous insects is achieved mainly <strong>by</strong><br />
avoiding the use of selective insecticides, especially in overall cover-spray<br />
treatments (Katsoyannos, 1996a).<br />
2.6. The Citrus Flower Moth, Prays citri<br />
The citrus flower moth Prays citri usually completes three generations in Greece<br />
whereas development time is estimated to range from 15 to 19 days in the region of<br />
Achaia-Peloponnese (Buchelos et al., 1963; Tzanakakis & Katsoyannos, 2003).<br />
The adults of the first generation appear in August <strong>and</strong> those of the second<br />
generation in October–November. Maximum infestation on lemons is observed at<br />
the end of their main florescence whereas the next generations of the pest infest the<br />
flowers <strong>and</strong> fruits of the subsequent florescences of multiple-flowering lemon trees<br />
(Buchelos, Sueref, & Tsoka-Thanasoulopoulou, 1963). The major damage concerns<br />
the citrus flowers <strong>and</strong> the newly formed fruits <strong>and</strong> it is more severe in lemons <strong>and</strong><br />
citrons. In addition, serious damages have been reported on new overgraftings at<br />
warm regions in autumn (Tzanakakis & Katsoyannos, 2003).<br />
Control of the pest depends largely on cultural practices <strong>and</strong> methods directed<br />
against the adult moths, since the larvae mining within the flower tissues are not<br />
normally vulnerable to insecticides <strong>and</strong> insect pathogens.<br />
2.6.1. Sampling <strong>and</strong> Monitoring<br />
Monitoring of infestation is possible <strong>by</strong> sampling <strong>and</strong> examination of flowers <strong>and</strong><br />
newly formed fruits (Cavalloro & Protta, 1983). Synthetic sex pheromone Z-7-<br />
tetradecenal is available in the US for monitoring (Mineo, Mirabello, del Busto, &<br />
Viggiani, 1983; Benfatto, 1984) or mass-trapping (120 traps/ha) of males<br />
(Sternlicht, Barzakay, & Tamim, 1990).<br />
Although no correlation exists between trap catch <strong>and</strong> level of flower damage<br />
(Mineo et al., 1983; Benfatto, 1984) as males of overlapping generations of the<br />
pest are caught throughout the growing season, both samples <strong>and</strong> trap captures are<br />
taken into account for accurate timing of chemical application on citrus (mainly<br />
lemon <strong>and</strong> citron) when required.<br />
The threshold of flower damage <strong>by</strong> P. citri for chemical control is estimated at<br />
>50% of flowers infested whereas in the case of fruits when 3% are affected<br />
(Cavalloro & Protta, 1983). A percentage of 20–30% of healthy flowers is<br />
sufficient for a satisfying production in lemons (Katsoyannos, 1996b).<br />
2.6.2. Biological Control <strong>and</strong> Cultural Practices<br />
Prays citri has several natural enemies, principally parasitoids e.g. Ageniaspis<br />
fuscicollis (Dalman) subsp. praysincola Silvestri (Hymenoptera: Encyrtidae) <strong>and</strong><br />
Elasmus flabellatus Boyer de Fonscolombe (Hymenoptera: Eulophidae), which are<br />
not always effective in contoling the pest (Tzanakakis & Katsoyannos, 2003).
IPM OF CITRUS PESTS IN GREECE<br />
49<br />
In twice-flowering lemons, good control of P. citri can be obtained <strong>by</strong> forcing<br />
early flowering in spring <strong>and</strong> summer, before the adult flight peaks of the pest in<br />
each season are observed (Calabretta & Nucifora, 1985).<br />
2.6.3. Chemical Control<br />
Registered insecticides (active substances), which can be used against P. citri in<br />
Greece, include Bacillus thuringiensis var. aizawai (citron, grapefruit, lemon,<br />
m<strong>and</strong>arin, orange), B. thuringiensis var. kurstaki (citron, grapefruit, lemon,<br />
m<strong>and</strong>arin, orange), chlorpyrifos (grapefruit, lemon, m<strong>and</strong>arin, orange, pumelo),<br />
cypermethrin (grapefruit, lemon, m<strong>and</strong>arin, orange), flucythrinate (grapefruit,<br />
lemon, m<strong>and</strong>arin, orange), paraffin oil (grapefruit, lemon, m<strong>and</strong>arin, orange,<br />
pumelo) <strong>and</strong> petroleum oil (grapefruit, lemon, m<strong>and</strong>arin, orange) (Authorized Plant<br />
Protection Products Data Base of the Hellenic Ministry of Rural Development <strong>and</strong><br />
Food, 2008).<br />
2.6.4. Recommended IPM Strategies<br />
Regulation of flowering before the adult flight peaks of the pest in secondflowering<br />
lemons is recommended. Selective chemicals could be applied, if<br />
necessary, after monitoring of infestation <strong>by</strong> sampling of flowers <strong>and</strong> newly<br />
formed fruits.<br />
2.7. Thrips<br />
Thrips species infesting citrus in Greece include the greenhouse thrips Heliothrips<br />
haemorrhoidalis (Bouché) (Thysanoptera: Thripidae) (Katsoyannos, 1996a;<br />
Tzanakakis & Katsoyannos, 2003) <strong>and</strong> the Kelly’s citrus thrips Pezothrips<br />
kellyanus (Bagnal) (Thysanoptera: Thripidae) which was first recorded in<br />
Peloponnese (Korinthos) in 1981 (Zur Strassen, 1986; Palmer, 1987). The<br />
greenhouse thrips H. haemorrhoidalis infests mainly citron <strong>and</strong> lemon whereas the<br />
Kelly’s citrus thrips P. kellyanus infests mainly lemon <strong>and</strong> orange with grapefruit<br />
following <strong>and</strong> m<strong>and</strong>arin being almost invulnerable (except the m<strong>and</strong>arin variety<br />
Minneola (tangelo) in Chania-Crete) (Varikou, Tsitsipis, Alex<strong>and</strong>rakis, & Mound,<br />
2002).<br />
In samplings performed in Chania – Crete in spring 2003, P. kellyanus was the<br />
only thrips species collected in lemon <strong>and</strong> m<strong>and</strong>arin orchards <strong>and</strong> the most<br />
abundant one collected in orange <strong>and</strong> grapefruit orchards. Some Thrips spp. were<br />
also found on m<strong>and</strong>arin <strong>and</strong> grapefruit in lower numbers whereas Frankliniella<br />
occidentalis was a minor species found solely in m<strong>and</strong>arin samples (Varikou,<br />
2006).<br />
In general, thrips are considered as a minor pest of citrus causing qualitative<br />
damage (scarring or escharosis) of the fruits (Katsoyannos, 1996a; Varikou et al.,<br />
2002; Tzanakakis & Katsoyannos, 2003; Hellenic Ministry of Rural Resources <strong>and</strong><br />
Food, 2006, unpublished data).
50<br />
F. KARAMAOUNA ET AL.<br />
However, escharotic fruits due to the feeding of the Kelly’s citrus thrips reached<br />
70% of the total produce in Chania-Crete <strong>and</strong> they were rejected for export during<br />
the selection process at packaging in 2001 (Varikou, 2006). Baker et al. (2005)<br />
refer that feeding of Kelly’s citrus thrips on young <strong>and</strong> mature fruit causes scarring<br />
(halo), marking <strong>and</strong> rind bleaching which typically encircles the apex of the fruit in<br />
the immediate vicinity of the calyx.<br />
Heliothrips haemorrhoidalis is a polyphagous parthenogenetic species which can<br />
complete six generations on citron <strong>and</strong> overwinters as an adult on citrus trees <strong>and</strong><br />
on poaceous weeds. This is the reason why weed control <strong>by</strong> ploughing, in<br />
February, was recommended together with chemical applications in March <strong>by</strong><br />
Anagnostopoulos (1939).<br />
The Kelly’s citrus thrips P. kellyanus is arrhenotokous (Varikou, 2006) <strong>and</strong> is<br />
not known to breed on any indigenous plant species of the Mediterranean region<br />
except Citrus sp. (Webster, Cooper, & Mound, 2005a). However, P. kellyanus<br />
can use the pollen of plant species other than citrus as an extra food resource.<br />
Biology of P. kellyanus was first studied <strong>by</strong> Varikou, Tsitsipis, Alex<strong>and</strong>rakis,<br />
<strong>and</strong> Hoddle, (2009a) <strong>and</strong> it was found that its lower development threshold is<br />
10.2 o C <strong>and</strong> its thermal constant 204.6 day degrees [whereas 504 day degrees for<br />
H. haemorrhoidalis (Rivnay, 1935)]. Therefore the Kelly’s citrus thrips is present<br />
throughout the year in Crete (Chania) with its population increasing during citrus<br />
flowering in spring as pollen is essential for its reproduction <strong>and</strong> development in<br />
the citrus orchards (Varikou, 2006; Varikou, Tsitsipis, & Alex<strong>and</strong>rakis, 2009b).<br />
Lemon is the best host among citrus for the survival <strong>and</strong> maintenance of the<br />
thrips population due to the numerous flowerings during the year. Pezothrips<br />
kellyanus is mostly attracted <strong>by</strong> blue colour traps (compared to yellow <strong>and</strong> white)<br />
at the fruiting period but not during flowering or the rest of the year (Varikou,<br />
2006).<br />
Entomophagous arthropods of the Kelly’s citrus thrips have not been studied in<br />
Greece. A predatory mite, Iphiseius (Amblyseius) degenerans (Berlese)<br />
(Phytoseiidae), has been found in citrus orchards with high thrips populations in<br />
<strong>Italy</strong> but its efficacy to control the thrips has not been not proved (Conti et al.,<br />
2001). Hence, chemical control is applied at present.<br />
Registered insecticides (active substances) for the control of thrips in citrus in<br />
Greece include chlorpyrifos, fatty acid potassium salt <strong>and</strong> oxamyl (Authorized<br />
Plant Protection Products Data Base of the Hellenic Ministry of Rural<br />
Development <strong>and</strong> Food, 2008).<br />
2.8. Mite Pests<br />
Citrus are infested <strong>by</strong> a large number of mite species in Greece i.e. the tetranychids<br />
Panonychus citri (Koch) <strong>and</strong> Tetranychus urticae Koch (Tetranychidae) <strong>and</strong> the<br />
eriophyiids Aculops pelekassi (Keifer) <strong>and</strong> Aceria sheldoni (Ewing) (Eriophyidae),<br />
which can cause serious damage on fruit production when outbreaks of the<br />
population occur (Papaioannou-Souliotis, 1985, 1991, 1996; Papaioannou-Souliotis,<br />
Tsagarakou, & Dermatas, 1992). However, the damages <strong>by</strong> mites are usually
IPM OF CITRUS PESTS IN GREECE<br />
51<br />
occasional <strong>and</strong> locally restricted as the natural enemies maintain the pest numbers<br />
under economic injury level in the citrus orchards.<br />
Panonychus citri was first recorded on Citrus spp. in Greece in 1986<br />
(Emmanouel & Papadoulis, 1987). It exists throughout the year <strong>and</strong> can complete<br />
many generations but the population is high in spring <strong>and</strong> fall (Papaioannou-<br />
Souliotis et al., 1992; Emmanouel, Papadoulis, Karkazi, & Papadima, 1994).<br />
Tetranychus urticae was first recorded in the country in 1962 (Pelekassis, 1962).<br />
Its population densities are higher during summer whereas in citrus orchards near<br />
the coast it is present throughout the year (Papaioannou-Souliotis, 1995).<br />
Aculops pelekassi was first found in 1958 <strong>and</strong> since then its presence is frequent<br />
all over the country (Papaioannou-Souliotis, 1985; Papaioannou-Souliotis, Ragusa<br />
di Chiera, & Tsolakis, 1996). It is active during mild winters <strong>and</strong> can develop more<br />
than five generations per year. In population outbreaks it can cause up to 60% loss<br />
of yield (Papaioannou-Souliotis, 1985). Aceria sheldoni has been found in all<br />
Greek citrus-growing regions, causing damage mainly in lemons, which can be<br />
significant only during years with high population (Papaioannou-Souliotis, 1985).<br />
Sampling for monitoring infestation involves collection of leaves <strong>and</strong> counting the<br />
number of mites.<br />
2.8.1. Biological Control <strong>and</strong> Cultural Practices<br />
Many phytoseiid predatory species are found in citrus orchards such as Euseius<br />
stipulatus (Athias-Henriot), Typhlodromus athenas Swirski <strong>and</strong> Ragusa,<br />
Amblyseius <strong>and</strong>ersoni (Chant) <strong>and</strong> Iphiseius degenerans Berlese. Euseius<br />
stipulatus is the most frequent phytoseiid predator <strong>and</strong> is the majority (80%) of the<br />
phytoseiid population in citrus groves (Papaioannou-Souliotis, 1991). Moreover it<br />
does not diapause <strong>and</strong> all the developmental stages may be present during winter<br />
(Papaioannou-Souliotis, Tsagkarakou, & Nomikou, 1997).<br />
Generalist predators like E. stipulatus can control the phytophagous mite<br />
populations at low densities (McMurtry, Morse, & Johnson, 1992) <strong>and</strong> especially<br />
the tetranychids when other food resources (e.g. pollen) are also available for their<br />
good development (Bouras & Papadoulis, 2005). Collection of the infested fruits is<br />
a practice which may decrease the population of mites.<br />
2.8.2. Chemical Control<br />
Low toxicity selective acaricides are used to control P. citri with applications in<br />
spring (when the first symptoms appear) <strong>and</strong> late October. The number of<br />
applications depends on the acaricide but more than two applications per year are a<br />
common practice (Papaioannou-Souliotis, 1985; Papaioannou-Souliotis, 1991;<br />
Papaioannou-Souliotis et al., 1992). Selective acaricides can be applied against A.<br />
pelekassi in summer (beginning of June) <strong>and</strong> autumn (mid September to mid<br />
November) <strong>and</strong> against A. sheldoni in spring <strong>and</strong> at the beginning of June<br />
(Papaioannou-Souliotis, 1985).
52<br />
F. KARAMAOUNA ET AL.
IPM OF CITRUS PESTS IN GREECE<br />
53<br />
Registered acaricides (active substances) for control of citrus mite pests include<br />
acrinathrin (P. ulmi), azocyclotin (P. ulmi <strong>and</strong> eriophyiids), clofentezine (P. ulmi),<br />
dicofol (all species), etoxazol (tetranychids), fenazaquin (tetranychids), fenbutatin<br />
oxide (all species), fenpyroximate (P. ulmi), paraffin oil (all species), petroleum oil<br />
(eriophyiids), propargite (tetranychids), pyridaben (P. ulmi), tebufenpyrad<br />
(tetranychids) <strong>and</strong> white oil (eriophyiids) (Authorized Plant Protection Products<br />
Data Base, Hellenic Ministry of Rural Development <strong>and</strong> Food, 2008).<br />
2.8.3. Recommended IPM Strategies<br />
Usually the phytoseiid predators (mainly E. stipulatus) keep the tetranychid mites<br />
at low populations on citrus. Monitoring of the mite population in citrus groves is<br />
very important for the early detection of mite infestation <strong>and</strong> hence the limited use<br />
of acaricides. Furthermore the use of selective acaricides highly contributes to<br />
conservation of the phytoseiid predatory mites.<br />
3. ARTHROPOD IPM IN CITRUS THROUGHOUT THE YEAR<br />
Following the IPM strategies recommended for each citrus insect pest separately,<br />
the outline of an overall IPM programme referring to these pests throughout the<br />
year is presented in Table 2 (Lykouressis, 1991; Katsoyannos, 1996a;<br />
Katsoyannos, 1996b; Alex<strong>and</strong>rakis et al., 2001).<br />
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3<br />
BIOLOGICAL CONTROL IN CITRUS IN SPAIN: FROM<br />
CLASSICAL TO CONSERVATION BIOLOGICAL<br />
CONTROL<br />
JOSEP ANTON JACAS 1 AND ALBERTO URBANEJA 2<br />
1 Universitat Jaume I (UJI), Unitat Associada d’Entomologia Agrícola<br />
UJI-IVIA, E-12071 Castelló de la Plana, Spain<br />
2 Institut Valencià d’Investigacions Agràries (IVIA), Unitat Associada<br />
d’Entomologia Agrícola UJI-IVIA, E-46113 Montcada, Spain<br />
Abstract. The status of citrus pest management in Spain <strong>and</strong> of biological control, including classical<br />
biological control strategies, is reviewed. The augmentative versus inoculation-based control, <strong>and</strong> the use<br />
of invertebrate biological control agents in citrus orchards <strong>and</strong> nurseries are described. Fortuitous <strong>and</strong><br />
conservation biocontrol strategies, as well as exploitation of resident species, either native or naturalized,<br />
are discussed. Pesticide side-effect testing on natural enemies, presence of alternative hosts <strong>and</strong> use of<br />
banker plants are described, together with ground cover mangement strategies.<br />
1. INTRODUCTION<br />
Spain is one of the largest producers of citrus for the fresh market worldwide<br />
(5,129,110 Mg in 2004; MAPA, 2007), mainly oranges, m<strong>and</strong>arins <strong>and</strong> lemons.<br />
Many potential pests are kept under excellent or satisfactory natural control <strong>by</strong> either<br />
exotic or indigenous natural enemies [e.g. Panonychus citri (McGregor) (Acari:<br />
Tetranychidae) <strong>by</strong> Euseius stipulatus (Athias-Henriot) (Acari: Phytoseiidae)] (Table<br />
1). Exotic biological control (BC) agents were imported during the last century into<br />
Spain following classical (= inoculative) BC programs <strong>and</strong> are now naturalized in<br />
our country [e.g. Rodolia cardinalis (Mulsant) (Coleoptera: Coccinellidae)] (Table<br />
2). However, the fact that most of Spanish citrus production goes to the fresh market<br />
(84.1%; MAPA, 2007) has important consequences on the status of some citrus<br />
pests which directly damage the fruit. Because these species are subjected to<br />
cosmetic thresholds, which are commonly very low (Hare, 1994), BC is considered<br />
A. <strong>Ciancio</strong>, K.G. Mukerji (eds.), Integrated Management of Arthropod Pests<br />
<strong>and</strong> Insect Borne Diseases, Integrated Management of Plant Pests <strong>and</strong> Diseases 5,<br />
DOI 10.1007/978-90-481-8606-8_3, © Springer Science+Business Media B.V. 2010<br />
61
62<br />
J.A. JACAS & A. URBANEJA<br />
insufficient on a limited, but important, number of pests, such as scales [e.g.<br />
Aonidiella aurantii (Maskell) (Hemiptera: Diaspididae)] or spider mites<br />
(Tetranychus urticae Koch) (Acari: Tetranychidae). Furthermore, because of the<br />
quarantine pest status of the Mediterranean fruit fly, Ceratitis capitata (Wiedemann)<br />
(Diptera: Tephritidae), thresholds are nil for fruit exported to C. capitata-free<br />
countries (Jacas, Palou, Beitia, & del Rio, 2008). Hence efforts to improve the BC of<br />
these species are underway. On the one h<strong>and</strong>, classical BC is a very powerful tool<br />
against exotic pests of an exotic crop such as citrus is in the Mediterranean basin,<br />
<strong>and</strong> this is one of the reasons why this type of BC has been so widely used in the<br />
region (Jacas, Urbaneja, & Viñuela, 2006). In recent years, though, concerns about<br />
the potential non-target effects of these exotic species on indigenous food webs have<br />
arisen worldwide (Lenteren, van Bale, Bigler, Hokkanen, & Loomans, 2006; Lynch<br />
& Thomas, 2000; Lookwood, Howarth, & Purcell, 2001; Stiling, 2004) <strong>and</strong> citrus is<br />
not an exception (Michaud, 2002).<br />
Table 1. Status of citrus pests in Spain <strong>and</strong> its relation to biological control (BC).<br />
Pest species<br />
Natural<br />
control a Key mortality factor b BC<br />
strategy c<br />
Icerya purchasi E Imported NE C<br />
Insulaspis gloverii E Imported NE C<br />
Aleurothrixus floccosus S Imported NE C<br />
Ceroplastes sinensis S Climate-Native NE C<br />
Chrysomphalus dyctiospermi S Native NE C<br />
Coccus hesperidium S Climate-Native NE C<br />
Panonychus citri S Native NE C<br />
Phyllocnistis citrella S Imported NE C<br />
Planococcus citri S Imported NE A<br />
Saissetia oleae S Climate-Native NE C<br />
Aonidiella aurantii I Native & imported NE A<br />
Aphis gossypii I Native & imported NE C, A<br />
Aphis spiraecola I Native & imported NE C, A<br />
Ceratitis capitata I Native & imported NE I, C<br />
Cornuaspis beckii I Native & imported NE C<br />
Parlatoria perg<strong>and</strong>ii I Native & imported NE C<br />
Tetranychus urticae I Indigenous NE C, A<br />
Toxoptera aurantii I Native & imported NE C, A<br />
a E: excellent; S: satisfactory; I: insufficient.<br />
b NE: natural enemies.<br />
c C: Conservation; A: augmentation; I: inoculation.<br />
A European Union (EU)-harmonized legislation on Invertebrate Biological<br />
Control Agents (IBCA) is expected to change the current situation of import <strong>and</strong><br />
release of exotic IBCAs in the EU. As a consequence, classical BC will probably<br />
lose its prevalence in the European citrus industry in favor of other BC strategies<br />
focused on existing IBCAs (either indigenous or naturalized) <strong>and</strong> their management.
CLASSICAL AND CONSERVATION BIOCONTROL<br />
63<br />
In this scenario both augmentative <strong>and</strong> conservation strategies aimed at increasing<br />
the impact of these natural enemies on citrus key pests will become the cornerstone<br />
of future Integrated Pest Management (IPM) in Spain.<br />
Table 2. Classical BC Programs developed in Spain against citrus pests.<br />
Target pest Year Natural enemy Establishment Success a<br />
Diaspididae 1908 Rhyzobius lophanthae Yes P<br />
C. dictyospermi 1936 Comperiella bifasciata No –<br />
Icerya purchasi 1922 Rodolia cardinalis Yes C<br />
1997 Cryptochaetum iceryae No –<br />
Saissetia oleae
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J.A. JACAS & A. URBANEJA<br />
2. THE ORIGINS: CLASSICAL BIOLOGICAL CONTROL IN CITRUS<br />
Classical BC has been profusely practiced in Spanish citrus orchards (Jacas et al.,<br />
2006). Up to 20 programs have been developed during the last century (Table 2).<br />
Citrus are an imported crop group in the Mediterranean basin <strong>and</strong> most of the pest<br />
species associated with them originate from Australasia, the area of origin of citrus.<br />
These are the typical conditions for pests to become the target of classical BC<br />
programs (Barbosa & Segarra-Carmona, 1993). Therefore, this strategy has been<br />
repeatedly applied not only in Spain, but in most Mediterranean countries (e.g. Cohen,<br />
1975; Garrido & Ventura, 1993; Katsoyannos, 1996), as well as in most other citrus<br />
growing areas under Mediterranean climate, such as California (UC, 1991), Australia<br />
(Smith, Beattie, & Broadley, 1997) or South Africa (Charleston et al., 2003).<br />
Scales are predominant among the target pests (Table 2) <strong>and</strong> this can not be<br />
considered an accident. Coccoidea represent 50.0% (n = 8) of them, <strong>and</strong> Homoptera<br />
as a whole represent 81.3% (n = 13). Well-protected insects, such as most<br />
homopterans, <strong>and</strong> those presenting concealed ways of life, like leaf miners, borers,<br />
etc. are often more likely to be successfully amenable <strong>by</strong> BC than free living ones<br />
(Hall & Bennett, 1994; Hespenheide, 1991; Khan, Overholt, & Ng’eny-Mengech,<br />
2003; Knipling, 1995). This could partly explain why the citrus leaf miner,<br />
Phyllocnistis citrella Stainton (Lepidoptera: Gracillariidae), ranks first, together with<br />
the Mediterranean fruit fly, or Medfly, C. capitata, according to the number of<br />
natural enemies introduced against each of them (n = 6).<br />
Whereas the Medfly is considered one of the world's most damaging fruit pests<br />
(IAEA, 2003; White & Elson-Harris, 2004), P. citrella is considered a secondary<br />
citrus pest. The case of this leaf miner can be considered a paradigm. As in similar<br />
situations (Michaud, 2002), the appraisal of urgency when P. citrella was detected in<br />
Spanish citrus orchards in 1993 prompted funding agencies to prioritize BC projects<br />
based on the rearing <strong>and</strong> release of imported natural enemies. Therefore, P. citrella<br />
became an automatic target for the classical BC approach without a critical evaluation<br />
if such an approach was useful. Pre-introduction studies (Lenteren & Woets, 1988;<br />
Barbosa & Segarra-Carmona, 1993; FAO, 1996; EPPO, 1999, 2000) were very limited<br />
(Urbaneja, Llácer, Tomás, Garrido, & Jacas, 2000; Urbaneja, Llácer, Garrido, & Jacas,<br />
2003) <strong>and</strong> 6 different parasitoids (Table 2), were introduced in less than 5 years. The<br />
host specific A. citricola successfully established on the Canary Isl<strong>and</strong>s, but from the<br />
remaining eulophids, only C. phyllocnistoides finally succeeded in establishing on the<br />
mainl<strong>and</strong> (Karamaouna et al., 2009).<br />
Although the introductions of exotic natural enemies focused on C. capitata<br />
began in 1931 (Servicio Fitopatológico Agrícola, 1933), no success has been<br />
achieved so far. A classical BC program against this pest is being carried out at<br />
present (Jacas et al., 2006) <strong>and</strong> both Fopius arisanus (Sonan) <strong>and</strong> Diachasmimorpha<br />
longicavdata (Ashmead) (Hymenoptera: Braconidae) will be probably released from<br />
quarantine confinement during 2010.<br />
Success has been higher for introductions aimed at regulating homopteran pests<br />
(Table 2). In fact, some of these natural enemies, like Rodolia cardinalis (introduced<br />
against I. purchasi), Cales noacki Howard (Hymenoptera, Aphelinidae) [imported in<br />
1971 against Aleurothrixus floccosus (Maskell) (Hemiptera: Aleyrodidae)] <strong>and</strong>
CLASSICAL AND CONSERVATION BIOCONTROL<br />
65<br />
Lysiphlebus testaceipes (Cresson) (Hymenoptera, Braconidae) [introduced in 1977<br />
against Aphis gossypii Glover <strong>and</strong> A. spiraecola Pagenstecher (Hemiptera:<br />
Aphididae)], are considered nowadays key natural enemies in Spanish citrus<br />
orchards (Urbaneja et al., 2008).<br />
3. AUGMENTATION VERSUS INOCULATION<br />
A few IBCAs primarily introduced in classical BC programs, namely the parasitoids<br />
Aphytis melinus DeBach (Hymenoptera: Aphelinidae) <strong>and</strong> Leptomastix dactylopii<br />
(Howard) (Hymenoptera: Encyrtidae) <strong>and</strong> the predator Cryptolaemus montrouzieri<br />
Mulsant (Coleoptera: Coccinellidae) failed to satisfactorily establish in Spain <strong>and</strong><br />
consequently do not usually reach numbers high enough to naturally regulate their<br />
target pests below economic thresholds (Table 2).<br />
Table 3. IBCAs used in augmentative BC strategies in Spanish citrus orchards <strong>and</strong> nurseries.<br />
Natural enemy Target pest Strategy<br />
Cryptolaemus<br />
montrouzieri<br />
Leptomastix<br />
dactylopii,<br />
Anagyrus<br />
pseudococci<br />
Aphytis<br />
melinus<br />
Neoseiulus<br />
californicus,<br />
Phytoseiulus<br />
persimilis<br />
Phytoseilus<br />
persimilis<br />
Planococcus<br />
citri<br />
Planococcus<br />
citri<br />
Aonidiella<br />
aurantii<br />
Panonychus<br />
citri,<br />
Tetranychus<br />
urticae<br />
Tetranychus<br />
urticae<br />
From end of April – July, if gravid females are<br />
present, release 3–10 individuals per tree<br />
Repeat at 2–3 week intervals.<br />
From May – July, when third instar nymphs <strong>and</strong><br />
young females are present, release 10–20<br />
individuals per infested tree<br />
Repeat at 2–3 week intervals<br />
From the end of winter, if parasite susceptible<br />
stages (NII, males <strong>and</strong> young females) are present,<br />
release 50–150 ⋅ 10 3 wasps/ha in 5 – 8 releases, 15<br />
days apart from each other<br />
In severely infested orchards, releases should be<br />
combined with petroleum spray oils a .<br />
In nurseries, hot spot releases of 10 – 30 individuals<br />
per infested young tree b .<br />
Hot spot releases of 100 – 500 individuals per tree<br />
when economic threshold (20% occupied leaves) is<br />
exceeded c .<br />
a Summer releases should be carefully considered due to hot temperatures <strong>and</strong> low relative humidity.<br />
Releases after summer are only recommended in orange orchards.<br />
b<br />
Against P. citri, only recommended in nurseries if Euseius stipulatus is not present.<br />
c Experimental strategy under development.
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Since the cost of production of these natural enemies is relatively low, the current<br />
use of these IBCAs involves augmentative releases against their respective target pests<br />
(Table 3). These strategies are also in use in other Mediterranean countries<br />
(Katsoyannos, 1996), as well as in areas with a similar climate, such as Australia,<br />
California, or South Africa (Charleston et al., 2003; UC, 1991; Smith et al., 1997).<br />
As shown in Table 3, augmentative releases include both exotic <strong>and</strong> native<br />
natural enemies. Consistent with latest trends in EU agriculture, which emphasizes<br />
the role of indigenous natural enemies, Anagyrus pseudococci (Girault)<br />
(Hymenoptera: Encyrtidae), a native parasitoid of the citrus mealybug, Planococcus<br />
citri Risso (Hemiptera: Pseudococcidae), has been recently studied <strong>and</strong> could<br />
successfully substitute the exotic L. dactylopii in the future (Campos & Martínez-<br />
Ferrer, 2003). Similarly, studies are in progress to establish conditions for using the<br />
native predatory mite Phytoseiulus persimilis Athias-Henriot (Acari: Phytoseiidae)<br />
against the two spotted spider mite, Tetranychus urticae Koch (Acari:<br />
Tetranychidae) another native mite which is considered a key pest for clementine<br />
m<strong>and</strong>arins in Spain (Aucejo, Gómez-Cadenas, & Jacas, 2004; Ansaloni, Pascual-<br />
Ruiz, Hurtado, & Jacas, 2008). Likewise, releases of Neoseiulus californicus<br />
(McGregor) (Acari: Phytoseiidae) <strong>and</strong> P. persimilis have also been proposed against<br />
the citrus mite, Panonychus citri, <strong>and</strong> T. urticae, respectively, in nurseries (Table 3)<br />
(Abad-Moyano, Pina, Pérez-Panadés, Carbonell, & Urbaneja, 2009).<br />
4. FORTUITOUS BIOLOGICAL CONTROL<br />
Anagyrus pseudococci is not the only example of an indigenous natural enemy<br />
having a significant impact on an exotic pest. Although such pests are usually the<br />
target of the Classical BC strategy, indigenous natural enemies can sometimes result<br />
in excellent BC, which is then called fortuitous BC.<br />
The native predator E. stipulatus provides a good example of such a situation in<br />
Spain. This species is the most abundant Phytoseiidae in Spanish citrus (Ferragut et al.,<br />
1988). If undisturbed, its populations are usually able to regulate Panonychus citri<br />
populations below their economic threshold (Ripollés, Marsá, & Martínez, 1995).<br />
Therefore E. stipulatus is considered as one of the most relevant natural enemies in<br />
Spanish citrus orchards <strong>and</strong> its conservation is a key factor for IPM success (Urbaneja<br />
et al., 2008). Most other indigenous natural enemies do not have such a dramatic<br />
impact on their host/prey pests (Table 1). However, both the increasing legal<br />
restrictions for importing exotic natural enemies into the EU (Bigler et al., 2005) <strong>and</strong><br />
the disappearance of many pesticides in the EU following the process of re-evaluation<br />
of all pesticide active ingredients under EU Directive 91/414/EEC, have lead to a<br />
renewed interest on these native species <strong>and</strong> their conservation (Table 1).<br />
5. THE CORNERSTONE: CONSERVATION<br />
Conservation biological control exploits resident, either native or naturalized,<br />
natural enemies. This strategy is especially useful in permanent ever-green crops<br />
(Barbosa, 1998; L<strong>and</strong>is, Wratten, & Gurr, 2000), such as citrus, where both pests<br />
<strong>and</strong> their natural enemies are active <strong>and</strong> abundant throughout the year (Garrido &
CLASSICAL AND CONSERVATION BIOCONTROL<br />
67<br />
Ventura, 1993). One of the most popular tactics used for the conservation of natural<br />
enemies in the Spanish citrus industry has been the use of pesticides with a reduced<br />
impact on beneficial arthropods <strong>by</strong> exploiting either their intrinsic or their ecological<br />
selectivities (Croft, 1990). The use of reservoir plants <strong>and</strong>, more recently, studies<br />
focused on both the management of the ground cover <strong>and</strong> the use of banker plants to<br />
enhance the performance of resident natural enemies are providing citrus growers<br />
new tools for implementing conservation BC in their orchards.<br />
5.1. The First Step: Pesticide Side-Effect Testing<br />
Citrus IPM has since long recognised the need for the evaluation of the impact of<br />
pesticides on the most relevant natural enemies. Pesticide side-effect testing was<br />
routinely done <strong>by</strong> Spanish researchers for many years for advisory purposes. As a<br />
consequence, in 2001, a database including around 270 records referred to 6<br />
important citrus IBCAs <strong>and</strong> 80 different pesticides was published (Jacas & García-<br />
Marí, 2001). The natural enemies were the parasitoids C. noacki, L. dactylopii, L.<br />
testaceipes <strong>and</strong> the predators C. montrouzieri, E. stipulatus <strong>and</strong> R. cardinalis. Some<br />
of the products tested up until that moment are no longer permitted in the EU<br />
whereas some new active ingredients have been registered. Therefore, there is a<br />
need for regularly updating that list. Pascual-Ruiz <strong>and</strong> Urbaneja (2006) recently<br />
revised the database.<br />
Results specifically dealing with acaricides have been recently published<br />
(Urbaneja et al., 2008). Products recommended for IPM in citrus orchards in the<br />
Region of Valencia have been listed in Table 4. When available, their residual<br />
toxicity on the selected IBCAs is provided. These products are effective against their<br />
target pests whereas their effects on IBCAs are usually low (Bacillus thuringiensis,<br />
Fenbutatin oxide, Hexithiazox, Mineral oils, Pirimicarb, Spinosad) <strong>and</strong>/or shortlasting<br />
(Mineral oils, Chlorpyrifos). In a few cases, some harmful products are<br />
allowed provided that ecological selectivity is exploited. This is the case of<br />
imidacloprid, which is prohibited from April till July to protect R. cadinalis which<br />
typically invades citrus orchards at that time.<br />
5.2. Alternative Hosts <strong>and</strong> Banker Plants<br />
There are two well-known examples of conservation BC in Spanish citrus orchards<br />
consisting of providing alternative hosts to natural enemies. One of them exploits<br />
Nerium ole<strong>and</strong>er L. (Gentianales: Apocynaceae), a bush native to the Mediterranean<br />
basin, as a reservoir for aphid natural enemies. Aphis nerii Boyer de Fonscolombe<br />
(Hemiptera: Aphidae) is a stenophagous aphid feeding on N. ole<strong>and</strong>er which can not<br />
survive on citrus. Because both A. nerii <strong>and</strong> citrus aphids, such as A. gossypii <strong>and</strong><br />
A. spiraecola, are attacked <strong>by</strong> the same guild of natural enemies (different aphidiine<br />
parasitoids <strong>and</strong> predators like syrphids, cecidomyids <strong>and</strong> coccinellids), Spanish<br />
citrus growers have long used N. ole<strong>and</strong>er to establish wind breaks <strong>and</strong> hedgerows<br />
in their orchards. However this strategy should not be used in lemon orchards
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J.A. JACAS & A. URBANEJA<br />
because N. ole<strong>and</strong>er hosts a key pest for this crop, the ole<strong>and</strong>er scale, Aspidiotus<br />
nerii (Bouché) (Hemiptera: Diaspididae).<br />
Table 4. Residual toxicity of active ingredients allowed under IP label in the Region of<br />
Valencia (CAPA, 2004). Classification according to the IOBC WG “Pesticides <strong>and</strong> Benefial<br />
Organisms” st<strong>and</strong>ards (1: harmless; 2: slightly harmful; 3: moderately harmful; 4: harmful).<br />
Active ingredient<br />
Target pests<br />
R. cardinalis<br />
C.<br />
montrouzieri<br />
E. stipulatus<br />
L. testaceipes<br />
L. dactylopii<br />
C. noacki<br />
Abamectin Mites, leaf miner 1 3–4 2–3 3–4<br />
Acetamiprid a Whiteflies, aphids, leaf miner<br />
Azadirachtin Leafminer 3–4 1 1 1 3–4<br />
B. thuringiensis Citrus moth 1 1 1 1 1 1<br />
Benfuracarb Aphids 1 2–3<br />
Buprofezin Diaspididae, whiteflies 1–2 3 1–2 1 1–2 1<br />
Chlorpyrifos Coccoidea, citrus moth, aphids 1–2 2 2 3 3 2–3<br />
Chlorpyrifos-methyl Medfly, coccoidea, citrus moth 1 1 3 3 3–4 1–2<br />
Clofentezine Mites 1 2 1–2 1<br />
Dicofol Mites 1 1–4 3–4 1 3–4 2<br />
Etoxazol a<br />
Mites<br />
Fenazaquin Mites 4 2 4 3<br />
Fenbutatin oxide Mites 1 2 1 1 1<br />
Fenperoximate a Mites<br />
Hexithiazox Mites 1 1 1<br />
Imidacloprid Leaf miner 4 2–3 1 4 3<br />
Mineral oil Mites, coccoidea, whiteflies 1 1–2 1–2 2 1 1–4<br />
Piridaben Mites 4 1<br />
Pirimicarb Aphids 1–2 2 1–2 1 1 1<br />
Pirimiphos-methyl Coccoidea, whiteflies 1–2 1–2 1–4 4 3–4<br />
Propargite Mites 4 1 2–3<br />
Pymetrozine a Aphids<br />
Pyriproxifen Coccoidea 4 4 1 1–2 2–3<br />
Spinosad Medfly 1 1 4<br />
Tebufenpyrad Mites 2<br />
a<br />
Products allowed under IP label whose side effects on citrus natural enemies are yet to be described.<br />
Source: Jacas <strong>and</strong> García Marí (2001), Pascual-Ruíz <strong>and</strong> Urbaneja (2006) <strong>and</strong> Urbaneja et al. (2008).<br />
A similar situation applies to Oxalis pes-caprae L. (Oxalidales: Oxalidaceae).<br />
This is an herbaceous plant indigenous of South Africa which was introduced long<br />
time ago into Spanish citrus orchards. It is an annual plant which produces a bulb<br />
that insures its survival. It usually dries during the dry Mediterranean summer, but<br />
reappears as the fall rainy season starts. Petrobia hartii (Ewing) (Acari:<br />
Tetranychidae) is an O. pes-caprae inhabitant which can not feed on citrus. Because<br />
this mite can serve as an alternative prey for the same Phytoseiid mites feeding on<br />
other phytophagous mites occurring on citrus, such as P. citri or T. urticae, the<br />
conservation of O. pes-caprae in citrus orchards was included in some citrus IPM
CLASSICAL AND CONSERVATION BIOCONTROL<br />
69<br />
guidelines (Aucejo et al., 2003). More recently, studies are underway to ascertain the<br />
usefulness of banker plants as a source of aphid parasitoids in citrus, using the same<br />
strategy already in use in protected crops (Calvo & Urbaneja, 2004). Barley plants<br />
infested with cereal-specific aphids, such as Rhopalosiphum padi (L.), parasitized <strong>by</strong><br />
aphidiine parasitoids, such as Aphidius colemani Viereck, are produced <strong>by</strong><br />
commercial insectaries <strong>and</strong> introduced into the orchards before citrus aphid<br />
populations peak during early spring. This strategy could prove very useful when<br />
grassy covers [e.g. Festuca arundinacea Schreb (Poales: Poaceae), see below]<br />
providing food to these specific aphids are also used.<br />
5.3. Ground Cover Management Strategies<br />
Spanish citrus orchards are quite commonly grown on bare soil <strong>by</strong> either use of<br />
herbicides or mechanical means. This is not the ideal situation <strong>and</strong> the use of a cover<br />
crop as an ecological infrastructure (Boller, Häni, & Poehling, 2004) is encouraged<br />
<strong>by</strong> IPM guidelines. However, little is still known about the fauna inhabiting this<br />
stratum in citrus <strong>and</strong> the ecological relationships occurring between the ground <strong>and</strong><br />
the tree arthropodofaunas. Therefore, the ground cover management is being<br />
investigated at this moment as a means of conserving ground-dwelling natural<br />
enemies <strong>and</strong> enhancing their impact on some citrus pests (top-down control), as well<br />
as a means of providing bottom-up control of these pests. This is the case of both<br />
T. urticae <strong>and</strong> C. capitata.<br />
Tetranychus urticae is a serious problem in clementine m<strong>and</strong>arins in the Eastern<br />
coast of Spain. Infestations downgrade fruit <strong>and</strong>, because T. urticae can feed on<br />
more than 900 plant species (Boll<strong>and</strong>, Gutiérrez, & Flechtmann, 1998), cover crop<br />
management can dramatically affect the dynamics of T. urticae populations on the<br />
trees. In 2003, a survey of the acarofauna associated to the most common weeds<br />
appearing in citrus orchards showed that Poaceae presented the lowest ratio<br />
T. urticae/Phytoseiidae from the 45 weed species studied (Aucejo et al., 2003).<br />
Therefore, a cover of Festuca arundinacea Schreb (Poales: Poaceae), a grass that<br />
had been previously selected as a citrus ground cover for other agronomic favorable<br />
characteristics, has been compared to a wild cover <strong>and</strong> to bare soil during the last 2<br />
years (2006–2007).<br />
The results obtained so far show that the F. arundinacea-sown cover has resulted<br />
in the lowest populations of T. urticae on the trees <strong>and</strong> could consequently be<br />
recommended to growers. The mechanisms explaining these results could be related<br />
both to a host-feeding specialization <strong>by</strong> T. urticae (bottom-up control) <strong>and</strong> to the<br />
composition of the beneficial acarofauna associated to the ground cover (top-down<br />
control), which resulted more diverse <strong>and</strong> balanced on both F. arundinacea <strong>and</strong> the<br />
trees grown on that particular cover than on both the wild cover <strong>and</strong> the bare soil<br />
systems (Aguilar-Fenollosa, Pascual-Ruiz, Hurtado-Ruiz, & Jacas, 2008, 2009). In<br />
addition to T. urticae, other citrus pests spend part of their life cycle on the ground<br />
cover, such as aphids, or in the soil, like C. capitata, which pupates in it. In recent<br />
years, different groups of ground-dwelling predators have been catalogued in<br />
Spanish citrus orchards (Monzó et al., 2005; Urbaneja et al., 2006). These studies
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showed that rove beetles (Coleoptera: Staphylinidae) were the most abundant-active<br />
group representing about 38.6% of the total number of predators collected, followed<br />
<strong>by</strong> spiders (Arachnida: Araneae) (28.9%), earwigs (Dermaptera) (18.0%), ground<br />
beetles (Coleoptera: Carabidae) (12.7%) <strong>and</strong> tiger beetles (Coleoptera: Cicindelidae)<br />
(1.8%). A recent study (Monzó, Urbaneja, Sabater-Muñoz, Castañera, 2007; Monzó,<br />
Mollá, Castañera, & Urbaneja, 2009) indicates that the wolf spider Pardosa cribata<br />
Simon (Araneae: Lycosidae), the most abundant ground-dwelling spider in the<br />
Valencian citrus orchards, could play an important role in controlling those pests.<br />
CONCLUSIONS<br />
Biological control has been <strong>and</strong> will definitively be an increasingly important part of<br />
citrus crop protection practices. Because of the present European limitations on the<br />
importation of exotic IBCAs, straightforward protocols to evaluate c<strong>and</strong>idate species<br />
are urgently needed. Simultaneously, studies focused on the role of indigenous<br />
IBCAs in the citrus agrosystem <strong>and</strong> the conservation of both native <strong>and</strong> naturalized<br />
natural enemies, have to be emphasized. Augmentative <strong>and</strong> conservation BC will<br />
probably play a gradually more important function in the Spanish citrus industry <strong>and</strong><br />
the first changes are already happening.<br />
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Karamaouna, F., Pascual-Ruiz, S., Aguilar-Fenollosa, E., Verdú, M. J., Urbaneja, A., & Jacas, J. A. (2009).<br />
Changes in predation <strong>and</strong> parasitism of the citrus leafminer Phyllocnistis citrella Stainton (Lepidoptera:<br />
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(Hymenoptera: Eulophidae). Biological Control, doi:10.1016/j.biocontrol.2009. 09.009.<br />
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Urbaneja, A., Llácer, E., Tomás, O., Garrido, A., & Jacas, J. A. (2000). Indigenous natural enemies<br />
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Agricultural Research.
4<br />
CITRUS INTEGRATED PEST MANAGEMENT<br />
IN ITALY<br />
LUCIA ZAPPALÀ<br />
Dipartimento di Scienze e Tecnologie Fitosanitarie,<br />
University of Catania, 95123 Catania, <strong>Italy</strong><br />
Abstract. Main insect pests of citrus in <strong>Italy</strong> are presented, with details on their biology <strong>and</strong> main natural<br />
enemies. They are the California red scale, Aonidiella aurantii, the Ole<strong>and</strong>er scale, Aspidiotus nerii, the<br />
Citrus mealybug, Planococcus citri, the Citrus leafminer, Phyllocnistis citrella <strong>and</strong> the Mediterranean fruit<br />
fly, Ceratitis capitata. Management of A. aurantii is generally based on integrated control strategies<br />
supported <strong>by</strong> a monitoring system through pheromone traps. Natural enemies include predatory beetles <strong>and</strong><br />
endoparasitoids. Aspidiotus nerii is controlled <strong>by</strong> predatory beetles <strong>and</strong> Aphelinid parasitoids. Management<br />
relies on pruning, chemical control <strong>and</strong> monitoring through sticky tapes. Several predators (spiders, true<br />
bugs, lacewings <strong>and</strong> ants) feed on P. citrella, with over 90 parasitoid species. Natural enemies of P. citri<br />
include predators <strong>and</strong> endoparasitoids, which provide satisfactory control. Ceratitis capitata is the main pest<br />
of citrus; biological control with parasitoids had limited success. Its populations are limited <strong>by</strong><br />
micro<strong>org</strong>anisms <strong>and</strong> occasional predators, cultural methods, chemicals <strong>and</strong> attractive traps. Management <strong>and</strong><br />
control of secondary pests of citrus, like whiteflies, some scales <strong>and</strong> moths, are also discussed.<br />
1. INTRODUCTION<br />
In <strong>Italy</strong> citrus are cultivated on around 170,,000 ha, the majority of which is<br />
represented <strong>by</strong> sweet orange (60%), followed <strong>by</strong> lemon (19%), clementine (13.8%),<br />
m<strong>and</strong>arin (6.1%) <strong>and</strong> minor species (bergamot, grapefruit, citron <strong>and</strong> chinotto)<br />
(1%).<br />
The pests reported on this crop are nearly 100 but among them only around 30,<br />
mainly sap-sucking species, may require control. In the last 30–40 years the picture<br />
of the main arthropod pests deeply changed. The major reason of this modification<br />
can be found in the repeated applications of large spectrum pesticides that altered<br />
the bio-ecological equilibrium of this complex agro-ecosystem. However, the<br />
changes are also related to the effect of modifications in cultural techniques<br />
(fertilization, use of phytoregulators, irrigation, pruning, weeding, new varieties,<br />
A. <strong>Ciancio</strong>, K.G. Mukerji (eds.), Integrated Management of Arthropod Pests<br />
<strong>and</strong> Insect Borne Diseases, Integrated Management of Plant Pests <strong>and</strong> Diseases 5,<br />
DOI 10.1007/978-90-481-8606-8_4, © Springer Science+Business Media B.V. 2010<br />
73
74<br />
L. ZAPPALÀ<br />
etc.) that modified the cultivated ecosystem. Besides, an additional cause of<br />
modifications in the citrus orchard fauna is represented <strong>by</strong> the accidental<br />
introduction of new exotic pests. Among these, the most significant in the last 30–40<br />
years have been Aphis spiraecola Patch, Aleurothrixus floccosus (Maskell),<br />
Dialeurodes citri (Ashmead), Parabemisia myricae (Kuwana), Coccus<br />
pseudomagnoliarum (Kuwana) <strong>and</strong> other scales [such as Aonidiella citrina (Coquet),<br />
Pseudococcus calceolariae (Maskell) <strong>and</strong> Unaspis yanonensis (Kuwana)],<br />
Phyllocnistis citrella Stainton, Pezothrips kellyanus (Bagnall) <strong>and</strong> the red spider<br />
mite Panonychus citri (McGregor). Recently (April 2008) a new record was added<br />
to the list of citrus pests in <strong>Italy</strong>: the Orange spiny whitefly Aleurocanthus spiniferus<br />
Quaintance (Porcelli, 2008). This species, which is included in the “EPPO A1 List of<br />
pests recommended for regulation as quarantine pests” <strong>and</strong> in the EU Annex II/A1:<br />
“Pests known not to occur in the EU, whose introduction into, <strong>and</strong>/or whose spread<br />
within, all EU Member States is prohibited, with reference to specific plants or plant<br />
products”, is a further example of fortuitous introduction of exotic species on citrus.<br />
The reasons of all these introductions are not easily explicable but they’re most<br />
probably related to increased commercial exchanges, as well as to continuous<br />
changes in climate. The flow of exotic arthropods towards the Mediterranean basin<br />
in general <strong>and</strong> <strong>Italy</strong> in particular is unceasingly active. There are several potential<br />
invasive species, among which the Brown citrus aphid Toxoptera citricidus (Kirk.),<br />
the most efficient vector of the Citrus Tristeza Virus, represents a real risk,<br />
considering its recent establishment in some limited areas of Spain <strong>and</strong> Portugal<br />
(Madeira isl<strong>and</strong> <strong>and</strong> Northern region). Other species that are most likely to be<br />
introduced or spread out in <strong>Italy</strong> are the whiteflies Aleurocanthus woglumi Ash<strong>by</strong>,<br />
Aleurodicus dispersus Russell, Aleuroclava jasmini (Takahashi) (which are all<br />
present in the Middle East); the psyllid Diaphorina citri Kuwayama (vector of the<br />
Greening disease <strong>and</strong> present in Saudi Arabia <strong>and</strong> in Madeira isl<strong>and</strong>); the scales<br />
Ceroplastes floridensis Comstock (recorded in the Middle East) <strong>and</strong> Chrysomphalus<br />
aonidum (L.) (up to now only occasionally reported on citrus in <strong>Italy</strong>), as well as the<br />
longhorned beetle Anoplophora chinensis (Forster) (reported in Northern <strong>Italy</strong> on<br />
other host plants).<br />
The introduction of exotic species is not only detrimental because of their direct<br />
damage but most of the time because of the measures adopted to control their<br />
populations, often chemical treatments, that may in fact disrupt comprehensive<br />
integrated control strategies carefully developed over the years. However, many of<br />
the newly introduced species have been the object of classical biological control<br />
programs with importation of natural enemies from the areas of origin of the pests<br />
<strong>and</strong> the majority of them achieved substantial results ensuring effective control.<br />
2. MAIN PESTS AND THEIR CONTROL METHODS<br />
In Italian citrus orchards the key arthropod pests are presently the California red<br />
scale Aonidiella aurantii (Maskell), the Ole<strong>and</strong>er scale Aspidiotus nerii Bouché (on<br />
lemon), the Citrus mealybug Planococcus citri (Risso), the Citrus leafminer<br />
P. citrella (on young trees <strong>and</strong> in nurseries), the Mediterranean fruit fly Ceratitis
CITRUS PEST MANAGEMENT IN ITALY<br />
75<br />
capitata (Wiedemann) <strong>and</strong> the Two spotted spider mite Tetranychus urticae (Koch)<br />
(on lemon) (Barbagallo, 2000). Together with these species, some others such as the<br />
Citrus green bug Closterotomus trivialis (Costa), the Cotton or Melon aphid Aphis<br />
gossypii (Glover), the Chaff scale Parlatoria perg<strong>and</strong>ii Comstock, the Olive black<br />
scale Saissetia oleae (Olivier), the Fig wax scale Ceroplastes rusci (L.) <strong>and</strong> the<br />
Leafroller Archips rosanus (L.), have been showing recrudescent infestations over<br />
the last decades.<br />
2.1. Aonidiella aurantii (Maskell)<br />
The armoured scale A. aurantii (Hemiptera: Diaspididae), commonly known as<br />
California red scale, is native to South-Eastern Asia (Southern China <strong>and</strong><br />
Indochinese peninsula) but is spread almost worldwide.<br />
The armour of the mature female is almost round in shape (1.6–2.1 mm), clear<br />
brown almost translucent with the nymphal exuviae located at the centre. Generally<br />
the scale appears reddish in colour because of the red body visible through the<br />
cover. The shield remains tightly attached to the substrate when the scales are<br />
moulting or reproducing. A characteristic, well developed, whitish ventral coating<br />
isolates the body of the female from the plant tissues. Before mating the body of the<br />
female is pear-shaped, pale yellow <strong>and</strong> its cover assumes a greyish colour; soon after<br />
mating, due to the production of eggs, the cephalothoracic portion of the body<br />
rapidly develops <strong>and</strong> reaches the apex of the abdomen. The crawlers that<br />
progressively emerge from under the female, move around to find a suitable place to<br />
settle <strong>and</strong> begin to produce a white cottony circular cover (“white cap” stage).<br />
Starting from the second instar, males begin to develop in a different way forming<br />
an elongated <strong>and</strong> usually clearer cover. The adult male (1.6–1.7 mm) emerges after<br />
four moults <strong>and</strong> is yellowish-orange, with some brown sclerified portions on the<br />
dorsal region.<br />
Figure 1. Aonidiella aurantii colonies on Tarocco orange.
76<br />
L. ZAPPALÀ<br />
Aonidiella aurantii is extremely polyphagous, it has been recorded on more than one<br />
hundred hosts including agricultural (almond, avocado, carob, grape, jujube, loquat,<br />
mango, mulberry, olive, peach, pear, walnut, etc.), forest (alder, conifer, eucalyptus,<br />
maple tree, oaks, etc.) <strong>and</strong> ornamental plants (acacia, aralia, araucaria, bougainvillea,<br />
boxwood, camellia, crossvine, dracaena, euonymus, magnolia, ole<strong>and</strong>er, palm, privet,<br />
etc.). However, its preferential host plants are citrus (Fig. 1), in decreasing susceptibility<br />
order: lemon, grapefruit, orange <strong>and</strong> m<strong>and</strong>arin, on which it can certainly be still<br />
considered as one of the key pests in arid <strong>and</strong> semiarid regions worldwide (Moreno &<br />
Luck, 1992; Franco, García–Mari, Ramos, & Besri, 2006; Grafton-Cardwell, 2006). This<br />
is related to the direct damage to the trees, due to the infestations on all aerial parts of the<br />
plant from which the scale sucks sap <strong>and</strong> inoculates toxic saliva causing leaf yellowing<br />
(Fig. 2), deformation <strong>and</strong> drop, dieback of twigs <strong>and</strong> limbs, cortical lesions on branches<br />
<strong>and</strong> trunk, sometimes with production of gum, but also mainly because of the<br />
commercial damage linked to fruit downgrading caused <strong>by</strong> the simple presence of instars<br />
on the peel (Walker, Zareh, & Arpaia, 1999).<br />
Figure 2. Leaf yellowing caused <strong>by</strong> Aonidiella aurantii on citrus.<br />
The general difficulty in chemically controlling armoured scales, the easy<br />
development of resistance <strong>by</strong> A. aurantii to chemical compounds (Forster, Luck, &<br />
Grafton–Cardwell, 1995; Grafton-Cardwell, Ouyang, Striggow, Christiansen, &<br />
Black, 2004; Martínez Hervás, Sots, & García–Marí, 2006) <strong>and</strong> the spread of<br />
integrated <strong>and</strong> <strong>org</strong>anic citriculture, led to the search for alternative control methods.
CITRUS PEST MANAGEMENT IN ITALY<br />
77<br />
Management of this pest is generally based on integrated control strategies<br />
supported <strong>by</strong> a monitoring system <strong>by</strong> means of pheromone traps. The captures allow<br />
identifying the flights of male scales, which correspond to the generations annually<br />
performed <strong>by</strong> the scale in the field, <strong>and</strong> also indicate which orchards or areas of the<br />
orchard have higher levels of scale population. The flight data together with the<br />
Degree-Days calculation, help to determine the right time for chemical or biological<br />
control. Pheromone traps have to be placed in the field in February-beginning of<br />
March. The sticky cards are then changed weekly <strong>and</strong> the pheromone dispensers<br />
monthly through October. Two to four pheromone traps per uniform 4-ha block are<br />
used, adding two traps for each additional 4 ha.<br />
Narrow range petroleum oil sprays can be used to reduce scale populations, with<br />
reduced negative effects on the complex of the natural enemies. Other commonly<br />
used chemicals, such as chlorpyrifos, imidacloprid or insect growth regulators<br />
(buprofezin, pyriproxifen), can negatively impact ladybeetle <strong>and</strong> lacewing<br />
populations <strong>and</strong> their use is therefore incompatible with a rational integrated<br />
management of the orchard. Pheromone traps, however, are not reliable predictors of<br />
red scale populations when insect growth regulators are used, since males are more<br />
sensitive than females to these compounds. In this case the traps may underestimate<br />
the scale population (Rill, Grafton–Cardwell, & Morse, 2007).<br />
The complex of natural enemies feeding on California red scale includes the<br />
predatory beetles Chilocorus bipustulatus (L.), C. kuwanae Silv., C. nigritus (F.),<br />
Exochomus quadripustulatus (L.), Rhyzobius lophanthae (Blaisdell) (Coleoptera:<br />
Coccinellidae), Cybocephalus rufrifrons Reitter (Coleoptera: Cybocephalidae), the<br />
dipteran Lestodiplosis aonidiellae Harris (Diptera: Cecidomyidae), <strong>and</strong> the mite<br />
Typhlodromus cryptus Athias-Henriot (Acari: Phytoseiidae). The scale is also<br />
controlled <strong>by</strong> the endoparasitoids Encarsia perniciosi (Tower) (Hymenoptera:<br />
Aphelinidae) <strong>and</strong> Comperiella bifasciata Howard (Hymenoptera: Encyrtidae), <strong>and</strong><br />
<strong>by</strong> the ectoparasitoids Aphytis chrysomphali (Mercet), A. lingnanensis Compere, A.<br />
melinus DeBach <strong>and</strong> A. proclia (Walker) (Hymenoptera: Aphelinidae).<br />
Figure 3. Aphytis melinus adult female.
78<br />
L. ZAPPALÀ<br />
Although numerous natural enemies are associated with California red scale <strong>and</strong><br />
their relative importance varies according to the differences in the climatic<br />
conditions as well as the host stage preferences, some of them are considered more<br />
effective <strong>and</strong> employed in biological control programs. In particular the aphelinid<br />
ectoparasitoid Aphytis melinus (Fig. 3) is the most commonly used biocontrol agent<br />
of A. aurantii in <strong>Italy</strong> as well as worldwide through augmentative releases (Furness,<br />
Buchanan, Ge<strong>org</strong>e, & Richardson, 1983; Moreno & Luck, 1992; Forster et al., 1995;<br />
Luck, Forster, & Morse, 1997; Rizqi, Nia, Abbassi, & Nadori, 2001; Rizqi,<br />
Bouchakour, Aberbach, & Nia, 2006). The technique consists in releasing about<br />
200,000 parasitoids/ha/year starting in February–March (when the average<br />
temperature is around 18°C or after the first captures of males on the pheromone<br />
traps) <strong>and</strong> following a bi-weekly interval. Half of the total amount of parasitoid<br />
adults should be released before mid-June, then the releases can be suspended for 1<br />
or 2 months (depending on the climatic conditions) when second <strong>and</strong> third instar<br />
scale are not available <strong>and</strong> then completed generally through mid-November.<br />
The effectiveness of biocontrol agents depends on careful monitoring <strong>and</strong> use of<br />
selective insecticides. Besides, a critical point is represented <strong>by</strong> the control of ants<br />
which can severely disrupt red scale parasites while protecting <strong>and</strong> maintaining this<br />
species <strong>and</strong> honeydew-producing pests, such as soft scales or mealybugs. In the last<br />
years some trials were carried out in Southern <strong>Italy</strong> (Tumminelli et al., 2000, 2006a;<br />
Mazzeo, Benfatto, Palmeri, & Scazziotta, 2004) which gave inconsistent results <strong>and</strong><br />
therefore the effectiveness of A. melinus releases has not been clearly demonstrated.<br />
The explanation of these results can be searched in the mutual relationship between the<br />
biology <strong>and</strong> behaviour of the parasitoid <strong>and</strong> its host, in the methodology of release, in the<br />
difficulty to involve uniform areas <strong>and</strong> in the low quality of the parasitoids used. In<br />
2005–2006 a further trial was carried out (Zappal à et al., 2008), trying to eliminate some<br />
of these elements of uncertainty, therefore conducting the experiment in a uniform<br />
integrated citrus orchard, releasing A. melinus locally produced <strong>by</strong> the insectary of the<br />
Regional Phytosanitary Services, regularly submitted to quality control tests (Zappalà<br />
Siscaro, Saraceno, Palmeri, & Raciti, 2006). Evenly distributed release points were used,<br />
according to a scheme supported <strong>by</strong> a parallel trial on the dispersal capacity of A. melinus<br />
(Palmeri, Campolo, Gr<strong>and</strong>e, Siscaro, & Zappalà, 2008). The data obtained suggest that<br />
A. melinus contributes to the control of California red scale infestations, but cannot be<br />
considered as the key solution, at least in Sicilian conditions. In any case the results<br />
obtained highlighted that the elimination of chemical treatments in the released plots as<br />
well as in the surroundings, restored a biological equilibrium ensuring a consistent<br />
presence of fundamental natural enemies (Zappalà et al., 2008).<br />
Further investigations presently focus on the evaluation of the actual role played<br />
<strong>by</strong> endoparasitoids, namely C. bifasciata, which was recovered several years after its<br />
first introduction (1988–1994). This species showed to be well adapted in Eastern<br />
Sicily where it has colonized a wide area, 50 km, on average, far away from the first<br />
release site. The presence of C. bifasciata both in <strong>org</strong>anic <strong>and</strong> conventionally<br />
managed orchards is of particular interest <strong>and</strong> could be of great help in the quick<br />
diffusion of the encyrtid, already successfully started, in all citrus growing areas of<br />
Southern <strong>Italy</strong> (Siscaro, Di Franco, & Zappalà, 2008). Future studies will also regard<br />
the interactions between A. aurantii, its natural enemies <strong>and</strong> the most common
CITRUS PEST MANAGEMENT IN ITALY<br />
79<br />
species of ants in Sicilian citrus orchards. Interesting hints could come from the<br />
evaluation of the effect of joint releases of predators, such as for example<br />
C. bipustulatus, which has an impressive “cleaning effect” on dense colonies, mostly<br />
on branches <strong>and</strong> trunk, <strong>and</strong> is less sensitive to high temperatures.<br />
2.2. Aspidiotus nerii Bouché<br />
Commonly known as Ole<strong>and</strong>er scale, A. nerii (Hemiptera: Diaspididae) is almost<br />
worldwide distributed on citrus <strong>and</strong> in the Mediterranean basin it normally<br />
completes 3 generations per year. It mainly overwinters as virgin female <strong>and</strong><br />
immature male on branches of various size. The reproduction is sexual or<br />
parthenogenetic <strong>and</strong> each female produces an average of 100 eggs with the<br />
parthenogenetic biotypes performing a lower fecundity. This scale insect is<br />
extremely polyphagous <strong>and</strong> attacks citrus (mainly lemon), acacia, asparagus, carob,<br />
ivy, jojoba, kiwi, mulberry, ole<strong>and</strong>er, olive, palm, peach, pear, plum.<br />
The armour of the female is pale brown in colour, about 1.5–2.5 mm in diameter,<br />
round shaped. The body of the insect is yellowish. The nymphal exuviae are yellow<br />
<strong>and</strong> located centrally or slightly laterally. The ventral shield is white <strong>and</strong> very thin.<br />
The pygidium has 3 pairs of lobes, the central ones have a sclerified basal region<br />
while the external ones are poorly developed; dorsal ducts are short <strong>and</strong> spiracles are<br />
not provided with gl<strong>and</strong>s.<br />
Male armour is slightly smaller, white <strong>and</strong> almost oblong in shape, 1–1.5 mm in<br />
length. The adult male (1 mm in length) has only one pair of wings, like all the other<br />
scales, <strong>and</strong> is characterized <strong>by</strong> a long aedeagus. It is yellow in colour with blackishbrown<br />
appendages.<br />
The pest infests branches, leaves <strong>and</strong> fruits. Heavy attacks may cause loss of<br />
vigour, deformation of infested plant parts, chlorotic spots on leaves <strong>and</strong> leaf drop.<br />
On the fruits the feeding sites of the scales remain green <strong>and</strong> do not develop<br />
normally while the rest of the rind changes colour at maturity <strong>and</strong> grows evenly.<br />
The Ole<strong>and</strong>er scale is controlled <strong>by</strong> the predatory beetles Chilocorus<br />
bipustulatus, Exochomus quadripustulatus, Rhyzobius lophanthae <strong>and</strong> Scymnus spp.<br />
(Coleoptera: Coccinellidae). The species is also parasitized <strong>by</strong> the Hymenoptera<br />
Aphelinidae Aphytis chilensis How., A. chrysomphali, A. diaspidis (How.), A.<br />
hispanicus (Mercet) <strong>and</strong> Encarsia citrina (Craw).<br />
Regular pruning represents an important tool in controlling this scale as well as<br />
all the other scales. Chemical control can be performed using mineral oils before the<br />
scale moves on the fruits <strong>and</strong>, in case of heavier infestations, the use of an IGR<br />
(buprofezin) can be considered. The timing of treatments is made harder <strong>by</strong> the<br />
absence of an efficient monitoring system. Pheromone traps were tried in the field<br />
but they were not commercially developed. A method which proved effective in<br />
monitoring the scale populations, <strong>and</strong> particularly in placing the chemical<br />
treatments, was based on wrapping sticky tape around 1-year-old branches that have<br />
both old <strong>and</strong> new wood <strong>and</strong> are infested <strong>by</strong> live female scales, in order to capture the<br />
crawlers as they emerge from the females <strong>and</strong> move across the twigs (Tumminelli,<br />
Perrotta, Raciti, & Colazza, 2006b). The economic threshold varies considerably,
80<br />
L. ZAPPALÀ<br />
depending on the market <strong>and</strong> crop yield, but it normally corresponds to 3–5% of fruits<br />
infested with more than 10 scales in the fall. If this threshold is exceeded at harvest,<br />
monitoring crawlers the following spring, together with visual inspection of fruit, may be<br />
a valid method to correctly place a treatment. This should be avoided at petal fall on the<br />
peak of crawlers of the first generation (around May) because it may increase fruit drop<br />
<strong>and</strong> be toxic to honeybees. It could instead be applied on the peak of crawlers of the<br />
second generation which normally takes place in July (Tumminelli et al., 2006b).<br />
2.3. Phyllocnistis citrella (Stainton)<br />
The Citrus leafminer (CLM), P. citrella (Lepidoptera: Gracillariidae), native to<br />
South-East Asia, has spread worldwide, throughout almost all citrus growing areas<br />
in the last decades (Hoy & Nguyen, 1997; CAB International, 2003; Grafton-<br />
Cardwell, Godfrey, Headrick, Mauk, & Peña, 2008). In <strong>Italy</strong> it was first reported in<br />
1994 (Benfatto, 1995).<br />
Adults are about 2 mm long with a wingspan of about 4 mm. They have narrow<br />
long fringed wings; the anterior pair is silvery <strong>and</strong> shining white with brown <strong>and</strong><br />
white markings as well as a distinct black spot on each wing tip. Hind wings are<br />
whitish <strong>and</strong> extremely slender, both costal <strong>and</strong> inner margins have long setae.<br />
Antennae are filiform <strong>and</strong> made of about 30 segments.<br />
The egg (0.35 × 2 mm) is lenticular <strong>and</strong> the chorion is smooth <strong>and</strong> transparent. The<br />
larvae are pale yellow from the first to the third instar with the last abdominal segment<br />
bifurcate. Their size is 1.7 – 2 × 0.3 – 0.4 mm. The fourth instar larva or prepupa is<br />
yellow in colour, cylinder shaped <strong>and</strong> without bifurcation on the last abdominal segment.<br />
It stops feeding but remains quite active. It forms a silken cocoon within the mine <strong>and</strong> as<br />
the silk dries the leaf curls over the pupal cell. The pupa is yellow to light brown, turning<br />
darker with age. It is characterized <strong>by</strong> the presence of a cephalic spine which is used to<br />
make an opening at the anterior of the chamber, to let the adult emerge. The last two<br />
abdominal segments are fused in the female pupa while they are distinct in the male.<br />
Figure 4. Phyllocnistis citrella larva <strong>and</strong> mine on a citrus leaf.
CITRUS PEST MANAGEMENT IN ITALY<br />
81<br />
Leafminers are most active from dusk to early morning. Soon after emergence<br />
the female emits a sex pheromone that attracts males. Females lay 30–70 eggs<br />
during their 2–12 days life span, deposited singly along the midrib on the lower<br />
surface of new tender terminal leaves. Eggs hatch within 2–3 days at 26–27°C;<br />
however, it may take up to 12 days at lower temperatures. Newly born larvae begin<br />
feeding immediately in shallow, winding mines under the leaf cuticle. As the larva<br />
increases in size, the mine becomes more visible because of the air that penetrates<br />
<strong>and</strong> because of the central frass trace within the mine (Fig. 4). Larvae molt 4 times,<br />
each larval stage lasting about 1 day, while the pupal stage lasts 7–10 days at 26°C.<br />
Mature larvae pupate within the mine inside a silken chamber under the rolled edge<br />
of the leaf. From egg to adult the life cycle takes about 15–17 days to complete at<br />
26°C <strong>and</strong> 70–80% humidity, but it may last up to 7 weeks depending on temperature<br />
<strong>and</strong> humidity conditions. Up to 13 generations per year occur in tropical areas. The<br />
population dynamics <strong>and</strong> the activities of the Citrus leafminer vary in relation to<br />
differences in climatic conditions <strong>and</strong> flushing of citrus trees. In <strong>Italy</strong> the spring<br />
flushing escapes P. citrella infestation since temperatures are not suitable for the<br />
leafminer development. The attacks of the pest occur during summer-fall.<br />
Several predators, mainly spiders, bugs, lacewings <strong>and</strong> ants, have been observed<br />
feeding on the pest (Browning & Peña, 1995). Besides, over 90 hymenopterous<br />
parasitoid species, belonging to the families Braconidae, Encyrtidae, Eulophidae,<br />
Eurytomidae, Eupelmidae <strong>and</strong> Pteromalidae have been reported (Heppner, 1993;<br />
Hoy & Nguyen, 1997; Schauff, Lasalle, & Wijesekara, 1998). Among these species,<br />
about 70 are considered as primary parasitoids <strong>and</strong> only 6 are classified as<br />
preferentially living on P. citrella. Indigenous natural enemies, mainly parasitoids,<br />
detected on the CLM never reached an effective control in all newly infested citrus<br />
areas, such as Florida (Hoy & Nguyen, 1997), Israel (Argov & Rössler, 1996), Spain<br />
(Garrido Vivas, 1995), Turkey (Uygun et al., 1996) <strong>and</strong> <strong>Italy</strong> (Barbagallo et al.,<br />
1998; Caleca & Lo Verde, 1998; Gi<strong>org</strong>ini, Pedata, & Viggiani, 1998).<br />
Since in the native areas of the leafminer the host-specific enemies represent the<br />
main biological mortality factor of the pest (Binglin & Mingdu, 1996; Morakote &<br />
Nanta, 1996; LianDe, MinSheng, Jin, & Qing, 1999), a classical biological control<br />
program has been started in 1995 in <strong>Italy</strong> <strong>by</strong> introducing exotic natural enemies.<br />
Three Hymenoptera parasitoids [Ageniaspis citricola Logvinovskaya (Encyrtidae),<br />
Quadrastichus sp. (now Quadrastichus citrella Reina & La Salle) <strong>and</strong> Citrostichus<br />
phyllocnistoides (Narayanan) (Eulophidae)] have been introduced, reared <strong>and</strong><br />
released. Moreover, in 1998 the Australasian ectoparasitoid Semielacher petiolatus<br />
(Girault) (Hymenoptera: Eulophidae) was recorded for the first time in <strong>Italy</strong>. The<br />
species probably spread naturally after its introduction in other countries of the<br />
Mediterranean basin (Mineo, Caleca, & Massa, 1998; Siscaro, Longo, Maugeri,<br />
Reina, & Zappalà, 1999a).<br />
Ageniaspis citricola (Fig. 5) is a poliembryonic koinobiont endoparasitoid of P.<br />
citrella eggs <strong>and</strong> young larvae (Edwards & Hoy, 1998; Zappalà & Hoy, 2004). The<br />
species shows several biological features which characterize effective parasitoids,<br />
such as host-specificity, high reproductive rate (more than 180 eggs/female, femalebiased<br />
sex ratio <strong>and</strong> short cycle), host discrimination capacity, high dispersal <strong>and</strong><br />
searching rate (Hoy & Nguyen, 1997; Zappalà & Hoy, 2004). Therefore, the
82<br />
L. ZAPPALÀ<br />
encyrtid A. citricola, native to Taiwan, Thail<strong>and</strong> <strong>and</strong> Vietnam, has been used in<br />
biological control programs in several citrus regions: Algeria, Argentina, Australia,<br />
Bahamas, Brazil, Cyprus, Colombia, Florida, Greece, Honduras, Israel, Louisiana,<br />
Morocco, Mexico, Oman, Peru, Syria, Spain, Texas, Tunisia, Turkey <strong>and</strong> Venezuela<br />
(Berkani & Mouats, 1998; Schauff et al., 1998; Siscaro, Longo, & Mineo, 2000).<br />
Figure 5. Ageniaspis citricola, ovipositing adult female.<br />
In <strong>Italy</strong>, the encyrtid has been introduced <strong>and</strong> reared since 1995 (Siscaro,<br />
Barbagallo, Longo, & Patti, 1997; Siscaro & Mazzeo, 1997). Nearly 15,000 adults<br />
have been released in Eastern Sicily <strong>and</strong> Calabria during 1996–2000 (Siscaro,<br />
Longo, & Mineo, 2000). The species was recovered in some coastal lemon orchards<br />
where it overwintered in 1998 (Siscaro et al., 1999a) <strong>and</strong> this strain, collected in the field,<br />
has been reared <strong>and</strong> released in the following years, although without any permanent<br />
establishment (Siscaro, Barbagallo, Longo, Reina, & Zappalà, 1999b). The encyrtid is,<br />
however, one of the major CLM antagonists in several countries (Argentina, Australia,<br />
Bahamas, Brazil, Canary Isl<strong>and</strong>s, Florida, Honduras, Louisiana <strong>and</strong> Venezuela), where it<br />
has permanently established. Therefore A. citricola appears to be climatically adapted to<br />
humid tropical <strong>and</strong> subtropical climates (Hoy & Nguyen, 1997).<br />
Laboratory observations have shown that the species, at the pupal stage, has a great<br />
resistance to low temperatures (5–10°C); adults survive longer at 10°C while individuals<br />
exposed to temperatures higher than 25°C die in less than 24 h. High mortality of adults<br />
at 25–35°C suggests that the parasitoid is unsuitable to the biological control of P.<br />
citrella in Mediterranean citrus orchards (Zappalà & Siscaro, 2004).<br />
Quadrastichus citrella is an ectoparasitoid of CLM second <strong>and</strong> third instar<br />
larvae. Its biological cycle lasts about 20 days at 20°C <strong>and</strong> R.H. > 80%. At the same<br />
temperature the adults survive up to 40 days (Argov & Rössler, 1998; Llácer,
CITRUS PEST MANAGEMENT IN ITALY<br />
83<br />
Urbaneja, Jacas, & Garrido, 1998). The parasitoid, native to China, Japan, Taiwan<br />
<strong>and</strong> Thail<strong>and</strong>, has been introduced in Morocco (Smaili, Afellah, Aarab, & Zrida,<br />
1999), Cyprus, Greece, Spain <strong>and</strong> Israel (Schauff et al., 1998; Kalaitzaki, 2004), with<br />
no evidence of establishment (Argov, 2000), except in Spain where the species<br />
temporarily established in the Valencia area (Vercher, García–Mari, Costa–Comelles,<br />
Marzal, & Villalba, 2003). In 1996 this eulophid was introduced in Southern <strong>Italy</strong> <strong>and</strong><br />
about 3,000 specimens were released in more than 30 sites. Although preliminary<br />
observations indicated that the ectoparasitoid seemed to have a good adaptability to<br />
Italian citrus areas (Longo & Siscaro, 1997), it has not overwintered in any release site<br />
(Barbagallo, Longo, Siscaro, Reina, & Zappalà, 2000).<br />
Citrostichus phyllocnistoides is reported as larval ectoparasitoid of P. citrella<br />
(Subba Rao & Ramamani, 1965; Bouček, 1988; Neale, Smith, Beattie, & Miles,<br />
1995). Nevertheless it has been recovered in India on Trioza obsoleta Buckton<br />
(Homoptera: Psyllidae) feeding on Diospyros melanoxylon (Roxb.) (Dash & Das,<br />
1997). Further studies (Massa, Rizzo, & Caleca, 2001; Massa & Rizzo, 2001; Lo<br />
Duca, Massa, & Rizzo, 2002) have shown that C. phyllocnistoides parasitizes also<br />
Lepidoptera Nepticulidae (Acalyptris minimella (Rebel) on Pistacia lentiscus L.,<br />
Stigmella sp. on Rubus ulmifolius Schott <strong>and</strong> an unidentified nepticulid on Salix alba<br />
L.). It prefers second <strong>and</strong> third instar CLM larvae both for ovipositing <strong>and</strong> host<br />
feeding, while first instar larvae are selected only for host feeding (Reina & Siscaro,<br />
2004). The female lays one or more eggs (up to 5), but only one will complete its<br />
development (Subba Rao & Ramamani, 1965). Its cycle lasts 12–13 days at 22–26°C<br />
(Ding, Li, & Huang, 1989). Sex ratio is female-biased, 80% of females is obtained<br />
from third instar larvae, while 70% of males from second instar larvae. The eulophid is<br />
reported on P. citrella in Afghanistan, China, India, Indonesia, Japan, Oman, Pakistan,<br />
South Africa, Sudan, Swazil<strong>and</strong>, Taiwan <strong>and</strong> Thail<strong>and</strong> (Schauff et al., 1998). It has<br />
been introduced in Australia, Cyprus, Greece, Israel (Schauff et al., 1998) <strong>and</strong> Spain<br />
(García-Marí et al., 2000). Its permanent establishment has been recorded in all these<br />
areas with the exception of Australia (Argov, 2000; García-Marí et al., 2000).<br />
Moreover, in Portugal the accidental immigration <strong>and</strong> establishment (ecesis) of this<br />
species was reported in 2003 (Gomes da Silva, B<strong>org</strong>es da Silva, & Franco, 2006).<br />
Figure 6. Semielacher petiolatus adult female.
84<br />
L. ZAPPALÀ<br />
In <strong>Italy</strong> C. phyllocnistoides was introduced in 1999 (Mineo & Mineo, 1999a) <strong>and</strong><br />
in the same year about 600 specimens were released in Western Sicily (Mineo,<br />
Mineo, & Sinacori, 2001). In 2000–2001 more than 3,000 specimens were released<br />
in Eastern Sicily (Conti, Raciti, Campo, Siscaro, & Reina, 2001). The eulophid was<br />
recovered in all the release sites (Conti et al., 2001) <strong>and</strong> also overwintered far from<br />
them (Mineo et al., 2001). Observations carried out in the following years showed<br />
its permanent establishment with a contribution to parasitization which increased<br />
from around 5% in 1999–2000 to almost 60% in 2001–2007.<br />
Semielacher petiolatus (Fig. 6) is a solitary ectoparasitic wasp which lays eggs<br />
on P. citrella second <strong>and</strong> third instar larvae (Fig. 7), although it frequently<br />
parasitizes also prepupae (Bouček, 1988; Argov & Rössler, 1998; Mineo & Mineo,<br />
1999b; Ateyyat, 2002; Lim & Hoy, 2005). It has been observed developing on<br />
alternative hosts, such as Diptera Agromyzidae Agromyza hiemalis Becker on<br />
Urtica spp., Chromatomyia horticola (Goureau) on Sonchus spp. <strong>and</strong> Liriomyza sp.<br />
on Merculiaris annua L. <strong>and</strong> Lepidoptera Cosmopterix pulchrimella Chambers<br />
(Cosmopterigidae) on Parietaria diffusa M. & K., Stigmella aurella (Fabr.)<br />
(Nepticulidae) on Rubus ulmifolius Schott <strong>and</strong> Dialectica scalariella Zeller<br />
(Gracillariidae) on Echium sp. (Massa & Rizzo, 2000; Massa et al., 2001).<br />
Figure 7. Semielacher petiolatus egg (yellow arrow) laid close to a CLM larva.<br />
The parasitoid, after various larval instars, pupates in host mines (Fig. 8) <strong>and</strong><br />
parasitized CLM larvae will not complete their development. The life cycle is<br />
completed in 10 days at 25°C. Host feeding was observed in the laboratory (Argov<br />
& Rössler, 1998). Semielacher petiolatus has been recovered on P. citrella in<br />
Australia (Bouček, 1988) <strong>and</strong> in Solomon Isl<strong>and</strong>s (Schauff et al., 1998). The<br />
eulophid has been introduced in Cyprus, Israel, Morocco, Oman, Syria, Tunisia,<br />
Turkey (Schauff et al., 1998), Egypt (Hamed, Reckhaus, Mahrous, Soliman, &<br />
Gassert, 1999), Greece (Michelakis, 1997) <strong>and</strong> Spain (García-Marí et al., 1997). In<br />
2003 adults of S. petiolatus were imported from <strong>Italy</strong> to Florida but after the<br />
evaluation in the quarantine facilities in order to verify the potential effectiveness of
CITRUS PEST MANAGEMENT IN ITALY<br />
85<br />
S. petiolatus as a natural enemy of the Citrus leafminer in Florida it was decided not<br />
to release it in the field (Lim & Hoy, 2005; Lim, Zappalà, & Hoy 2006). In <strong>Italy</strong> the<br />
parasitoid has been detected for the first time on P. citrella in 1998 (Mineo et al.,<br />
1998), performing interesting parasitism activity (Caleca, Lo Verde, Bl<strong>and</strong>o, & Lo<br />
Verde, 1998). Further observations have shown its spontaneous diffusion in all<br />
citrus orchards in Southern <strong>Italy</strong> (Viggiani, 2001). This record together with<br />
Algerian (Schauff et al., 1998) <strong>and</strong> Jordanian ones (Mineo, 1999), reveals its<br />
dispersal capability in Mediterranean citrus areas (Siscaro et al., 2000).<br />
Figure 8. Semielacher petiolatus larva (left) <strong>and</strong> pupa (right). The leaf cuticle has been<br />
removed to reveal the parasitoid instars.<br />
As reported for C. phyllocnistoides, also for S. petiolatus accidental<br />
immigration <strong>and</strong> establishment was observed in Portugal in 2003 where the<br />
parasitoid is now very frequently present (Gomes da Silva et al., 2006). In 1999–<br />
2000 S. petiolatus contribution to the total CLM biological control in <strong>Italy</strong> was<br />
around 90% (Mineo & Mineo, 1999b; Conti et al., 2001). In summer 2001 the<br />
eulophid was still the most efficient P. citrella parasitoid, showing an incidence on<br />
the total parasitization activity near 80%. Nevertheless during fall of the same year,<br />
the main biological control was also due to C. phyllocnistoides. In the following<br />
years the role of this last species greatly increased (up to 60%) being still more<br />
active in the final part of the CLM infestation season (September–October), while S.<br />
petiolatus is mainly active in early summer.<br />
Several indigenous Hymenoptera parasitoids belonging to the family Eulophidae<br />
have been obtained from samples collected in Italian citrus groves infested <strong>by</strong><br />
P. citrella. The main species were Cirrospilus pictus (Nees) <strong>and</strong> Pnigalio agraules<br />
(Walker) <strong>and</strong>, as observed in other Mediterranean citrus growing areas (Garrido
86<br />
L. ZAPPALÀ<br />
Vivas, 1995; Argov, Rössler, & Rosen, 1995), the incidence of the first one on the<br />
parasitization has reached 80–90% (Caleca et al., 1998; Caleca & Lo Verde, 1998;<br />
Conti et al., 2001). Moreover, the following species have been occasionally detected<br />
in Sicily: Apotetrastichus postmarginalis (Bouček), A. sericothorax (Szelényi),<br />
Asecodes delucchii (Bouček), A. erxias (Walker), Neochrysocharis formosa<br />
(Westwood) <strong>and</strong> Ratzeburgiola incompleta Bouček. Finally, other eulophids have<br />
been rarely recovered: Aprostocetus spp., Baryscapus sp., Chrysocharis pentheus<br />
(Walker), Cirrospilus diallus Walker, C. nr. lyncus (Nees), C. vittatus Walker,<br />
Diglyphus isaea (Walker) <strong>and</strong> Pnigalio soemius (Walker) (Viggiani & Gi<strong>org</strong>ini,<br />
1995; Benfatto, 1996; Caleca, Lo Verde, & Massa, 1996; Liotta, Peri, Salerno, Di<br />
Cristina, & Manzella, 1996; Caleca et al., 1998; Caleca & Lo Verde, 1998; Gi<strong>org</strong>ini<br />
et al., 1998; Lo Pinto & Salerno, 1998; Mineo, 1999; Conti et al., 2001).<br />
Starting from 1999 to 2002 the exotic eulophids C. phyllocnistoides <strong>and</strong><br />
S. petiolatus have progressively substituted almost all the indigenous parasitoids<br />
previously detected on P. citrella, inducing a decrease of their parasitism to less than<br />
one third of what had been recorded, up to 1998.<br />
The high degree of specificity reached <strong>by</strong> P. citrella parasitic complex represents<br />
an important element in the biological control of this pest. The data collected in the<br />
main Italian citrus growing areas from 1996 up to now reveal an activity of the<br />
parasitoids (including both parasitization <strong>and</strong> host feeding) that has grown from 32%<br />
(1996–1998) up to 65% in more recent years (Siscaro & Reina, 2005), mainly<br />
thanks to the biocontrol activity of the 2 exotic eulophids S. petiolatus <strong>and</strong> C.<br />
phyllocnistoides. These species permanently established in Sicilian citrus groves<br />
showing a contribution of 90% to the total parasitization (Siscaro, Caleca, Reina,<br />
Rizzo, & Zappalà, 2003). Besides, a seasonal alternation in their activity was<br />
highlighted: S. petiolatus parasitization is in fact mainly concentrated in the first<br />
months of CLM infestation (June–August), while C. phyllocnistoides activity is<br />
more intense in the second part of the season (September–October) (Siscaro et al.,<br />
2003).<br />
The establishment of the introduced eulophids is most likely related to the<br />
presence of alternative hosts (Massa et al., 2001; Massa & Rizzo, 2001; Lo Duca et<br />
al., 2002), <strong>and</strong> their seasonal alternation could be partly explained <strong>by</strong> the different<br />
biological <strong>and</strong> ecological attitudes the two species showed on hosts of native flora<br />
(Rizzo, 2003). Therefore it is important to maintain a rich biodiversity in citrus<br />
groves in order to provide alternative food <strong>and</strong> shelter to CLM parasitoids, mainly in<br />
winter <strong>and</strong> spring, when CLM populations are at their minimum levels.<br />
Biological control, together with cultural techniques based on reducing irrigation<br />
<strong>and</strong> fertilization with the aim of containing excessive vegetation, has proved<br />
effective in containing P. citrella infestations in adult citrus orchards. The situation<br />
is different on young <strong>and</strong> re-grafted trees, as well as in nurseries where damage<br />
caused <strong>by</strong> the leafminer may be more serious. In these cases chemical treatments can<br />
be applied using cytotropic or systemic insecticides, or insect growth regulators<br />
which, for their mode of action, should be employed sooner than the previous<br />
compounds. Mineral oils also have a repellent action on egglaying females <strong>and</strong> a<br />
reduced impact on the ecosystem. They can be used at a dose of 0.5–1 l/hl which<br />
protects the plants for 6–10 days, without rain, <strong>and</strong> the treatments must be applied
CITRUS PEST MANAGEMENT IN ITALY<br />
87<br />
sooner than the other larval insecticides in the infestation season (Siscaro &<br />
Zappalà, 2004).<br />
2.4. Planococcus citri (Risso)<br />
This mealybug (Hemiptera: Pseudococcidae), commonly known as Citrus mealybug,<br />
is reported as citrus pest in the Mediterranean basin together with five other<br />
mealybug species. It has uncertain origins, but recent findings on its main<br />
parasitoids indicate that it has spread from central Africa (Franco, Suma, B<strong>org</strong>es de<br />
Silva, Blumberg, & Mendel, 2004) <strong>and</strong> is now present almost worldwide.<br />
The adult female (1.6–3 mm long) has a convex body covered with a waxy<br />
secretion <strong>and</strong> is surrounded <strong>by</strong> 18 pairs of lateral filaments, with slightly increasing<br />
length from the head to the abdomen. Antennae <strong>and</strong> legs are well developed. A<br />
ventral circulus is present on the ventral part of the abdomen. The ovipositing<br />
female produces a white ovisac that covers the eggs. The light yellow crawlers are<br />
highly mobile.<br />
It is a very polyphagous species which can infest almost all species <strong>and</strong> varieties<br />
of citrus with a different degree of susceptibility (Franco et al., 2004), as well as<br />
several other agricultural <strong>and</strong> ornamental crops such as ficus, gardenia, jasmine,<br />
ole<strong>and</strong>er, persimmon, pothos, pittosporum, rhododendron, etc.<br />
It mainly overwinters as immature female but also younger instar nymph, which<br />
can be found in crevices on trunks <strong>and</strong> branches. It performs several generations per<br />
year (more than 5) <strong>and</strong> is favoured <strong>by</strong> warm <strong>and</strong> humid climate. Small colonies of<br />
the mealybug start settling in early summer, near the calyx of little fruits, in the<br />
contact points between them or, for some varieties, in the navel. High population<br />
levels are reached in late summer-fall. Several agronomic factors can favour the<br />
presence of P. citri, such as particularly dense <strong>and</strong> dark canopy, clusters of fruits,<br />
presence of navel, excess in nitrogen fertilization <strong>and</strong> irrigation. A very important<br />
role in the growth <strong>and</strong> dispersal of P. citri colonies is played <strong>by</strong> ants, which usually<br />
breed the mealybug, carrying it in good feeding sites in order to increase the<br />
production of honeydew which they feed on. Ants also protect P. citri from its<br />
natural enemies, thus disrupting biological control.<br />
Planococcus citri infestations can produce a reduction in plant growth <strong>and</strong> in<br />
fruits size, as well as fruit downgrading, caused <strong>by</strong> the presence of colonies with<br />
chlorotic areas surrounding the mealybug feeding sites <strong>and</strong> sooty mould developing<br />
on honeydew. High infestations can also cause defoliation, fruit splitting <strong>and</strong> fruit<br />
drop. Besides, some secondary pests such as the Honeydew moth Cryptoblabes<br />
gnidiella (Millière) (Lepidoptera: Pyralidae), may develop on fruits infested <strong>by</strong> the<br />
Citrus mealybug.<br />
Several species of indigenous natural enemies are reported, such as the predators<br />
Sympherobius spp. (Neuroptera: Hemerobiidae), Scymnus spp. (Coleoptera:<br />
Coccinellidae), Dicrodiplosis spp. (Diptera: Cecidomyiidae) <strong>and</strong> Leucopis spp.<br />
(Diptera: Chamaemyiidae), <strong>and</strong> the parasitoids Anagyrus pseudococci s.l. <strong>and</strong><br />
Leptomastidea abnormis (Girault) (Hymenoptera: Encyrtidae). They all actively<br />
contribute to the control of the Citrus mealybug, although this is essentially due to
88<br />
L. ZAPPALÀ<br />
the activity of the two encyrtids which can reach parasitization levels respectively of<br />
up to 60% A. pseudococci (Raciti, Barraco, & Conti, 2001) <strong>and</strong> 18–60% L. abnormis<br />
(Viggiani, 1974; Longo, 1985). The first species is already present in June, even<br />
though at very low densities, <strong>and</strong> it shows peaks of activity in August–September<br />
(Raciti et al., 2001).<br />
The control of P. citri represents a very good example of application of IPM<br />
strategies. Satisfactory results have been achieved with inoculative releases of the<br />
endoparasitoid Leptomastix dactylopii Howard (Hymenoptera: Encyrtidae). This<br />
species is native to Central America <strong>and</strong> was introduced in <strong>Italy</strong> for the first time in<br />
1955 for the biological control of P. citri (Zinna, 1960). Later, it was re-introduced<br />
in almost all Italian citrus growing regions (Longo, Mazzeo, & Siscaro, 1994).<br />
However, in the climatic <strong>and</strong> ecologic conditions of North-Mediterranean citrus<br />
growing areas, L. dactylopii is not able to overwinter <strong>and</strong> therefore needs to be<br />
reared <strong>and</strong> periodically inoculated in the field through releases replicated every year<br />
(Katsoyannos, 1996; Longo et al., 1994). The releases must be preceded <strong>by</strong> the<br />
localization of infested trees, on which 20–30 adult parasitoids per tree will be<br />
inoculated around May–June. In this period the average temperature is higher than<br />
15°C <strong>and</strong> the first young Citrus mealybug females start moving from the trunks to<br />
the fruits or the initial small colonies begin settling (Longo et al., 1994). The<br />
releases can be repeated, if necessary, in June–July up to a total of 2,000<br />
specimens/ha (Raciti et al., 2001). However, the encyrtid has proved effective in<br />
controlling the Citrus mealybug, reaching parasitization levels in some cases higher<br />
than 90% (Mineo & Viggiani, 1976; Longo & Benfatto, 1982; Spicciarelli,<br />
Battaglia, & Tranfaglia, 1994; Fronteddu, Basoni, Canu, Fancello, & Nanni, 2000).<br />
Other exotic species that were introduced to control the Citrus mealybug are the<br />
predators Cryptolaemus montrouzieri Mulsant <strong>and</strong> Nephus reunioni Fürsch<br />
(Coleoptera: Coccinellidae) <strong>and</strong> the parasitoid Coccidoxenoides perminutus Girault<br />
(Hymenoptera: Encyrtidae). Cryptolaemus montrouzieri was first introduced in <strong>Italy</strong><br />
in 1908 <strong>and</strong> established in Italian citrus orchards but in case of unfavourable<br />
climatic conditions or irrational chemical treatments its populations can be strongly<br />
reduced <strong>and</strong> need to be reintegrated <strong>by</strong> means of inoculative releases. Nephus<br />
reunioni was instead introduced in <strong>Italy</strong> in 1985 but didn’t manage to establish <strong>and</strong><br />
its predatory activity was unsufficient to control P. citri populations (Longo &<br />
Benfatto, 1987). The parasitoid C. perminutus established, but occurs in the field at<br />
very low densities (Franco et al., 2004).<br />
Pheromone traps may be used to monitor the pest population dynamics in the<br />
field but, given the inconsistent correlation between the number of captures <strong>and</strong> the<br />
levels of infestation on fruits (Franco et al., 2001; Franco, Gross, Silva, Dunkelblum,<br />
& Mendel, 2002), this technique should be joined <strong>by</strong> the direct observation of fruits<br />
(10 fruits on 10% of the trees) to verify the levels of infestation in relation to the<br />
economic threshold (5–10% of infested fruits).<br />
However, the traps, if placed early in May, are a very useful tool to detect the<br />
beginning of the mealybug activity in order to plan eventual releases of natural<br />
enemies after evaluating the presence of overwintering females on the trunk <strong>and</strong><br />
branches, identifying the infested trees to be used as release spots <strong>and</strong> evaluating the<br />
occurrence <strong>and</strong> the activity of ants. These may in fact protect honeydew producing
CITRUS PEST MANAGEMENT IN ITALY<br />
89<br />
pests from their natural enemies thus disrupting their control action (Delabie, 2001;<br />
Eubanks, Blackwell, Parrish, Delamar, & Hull-S<strong>and</strong>ers, 2002; Kaplan & Eubanks,<br />
2002). The negative role played <strong>by</strong> ants in biological control programs suggests to<br />
manage their populations using one of the various available techniques, including<br />
cultural methods such as canopy pruning to avoid contact with weeds <strong>and</strong> soil tillage<br />
to disturb their nests, as well as chemical or mechanical methods using insecticidetreated<br />
baits, sticky or insecticide-treated b<strong>and</strong>s placed around the trunk <strong>and</strong> ground,<br />
trunk or foliar treatments with insecticides (Tumminelli, Saraceno, & Conti, 1997;<br />
Benfatto, 1999; Franco et al., 2004). In Italian citrus orchards the most common ant<br />
species that are known to have interactions with honeydew-producing insects, thus<br />
potentially disrupting the control activity of their natural enemies, are Lasius alienus<br />
(Förster), Tapinoma nigerrimum (Nyl<strong>and</strong>er) <strong>and</strong> Camponotus nyl<strong>and</strong>eri Emery (La<br />
Pergola, Alicata, & Longo, 2008). Pheidole pallidula Nyl<strong>and</strong>er is also quite<br />
abundant in citrus orchards <strong>and</strong> although it is a typical terricolous species, it has<br />
been seen foraging on colonies of sapsucking insects (La Pergola, 2008).<br />
Chemical control of P. citri should be applied in case of high infestations, using<br />
IGRs, such as buprofezin, in summer-fall or, in the fall, <strong>org</strong>anophosphates such as<br />
chlorpyrifos-methyl. Good results can also be obtained with mineral oils.<br />
Present researches focus on the enhancement of the activity of native parasitoids<br />
(namely A. pseudoccocci s.l.) <strong>by</strong> using semiochemicals (Franco et al., 2008).<br />
2.5. Ceratitis capitata (Wiedemann)<br />
This species, commonly known as Mediterranean fruit fly, is widely distributed in<br />
Sub-Saharian Africa (from where it probably originated), in the Mediterranean basin<br />
(including France <strong>and</strong> the Balkans up to Hungary), in the Middle East, in Saudi<br />
Arabia, in Central <strong>and</strong> South America, in Western Australia <strong>and</strong> in Hawaii. In<br />
Germany it has been observed several times attacking fruit but it is not permanently<br />
established. In Mexico, Florida <strong>and</strong> California its occurrence has been faced through<br />
eradication programs, however hypothesis of permanent establishment have been<br />
formulated.<br />
The adult is 3.5–5 mm long, yellowish with brown tinge, especially on abdomen<br />
<strong>and</strong> legs. Eyes are reddish-purple <strong>and</strong> ocellar bristles are present. Male has a pair of<br />
bristles with enlarged spatulate tips next to the inner margins of the eyes. Thorax is<br />
creamy white to yellow, with characteristic pattern of black blotches. Light areas<br />
with very fine white bristles are present as well as humeral bristles. Scutellum is<br />
enlarged <strong>and</strong> shiny black. Abdomen is oval with fine black bristles scattered on<br />
dorsal surface <strong>and</strong> 2 narrow transverse light b<strong>and</strong>s on basal half. Ovipositor, when<br />
extended, is 1.2 mm long. Wings, usually held in a drooping position on live flies,<br />
are broad <strong>and</strong> hyaline with black, brown <strong>and</strong> brownish yellow markings. One<br />
longitudinal orange-yellowish b<strong>and</strong> crosses middle of wing, two similar transversal<br />
b<strong>and</strong>s are present on the caudal part of the wings.<br />
The egg is shiny white, elongate, slightly curved, tapering <strong>and</strong> 1 mm long, with<br />
micropylar region distinctly tubercular. The mature larva is 7–9 mm long,
90<br />
L. ZAPPALÀ<br />
yellowish-white, slender, elongate, tapering anteriorly. The pupa is reddish-brown,<br />
4.5 mm long. Some strains have pupae of different colour in the two sexes.<br />
The Mediterranean fruit fly is known to attack more than 260 different fruits,<br />
flowers, vegetables <strong>and</strong> nuts. Thin-skinned, ripe succulent fruits are preferred (apple,<br />
apricot, coffee, fig, Indian fig, loquat, peach, pear, persimmon, strawberries, etc.).<br />
Although it may be a major pest of citrus (Fig. 9), often it is a more serious pest of<br />
some deciduous fruits, such as peach, pear, <strong>and</strong> apple.<br />
Using the oviscapt the female lays eggs in clusters of 1–15 (in relation to the size<br />
of the fruit), about 2–5 mm deep under the skin of fruits. Oviposition may take from<br />
2 to 20 min. Although each female after oviposition normally labels the fruit with<br />
deterrent substances, several females may lay eggs in the same fruit <strong>and</strong> up to 80<br />
eggs may be found. This might be related to the decreased deterring efficacy on<br />
large fruits. One single female may lay as many as 22 eggs/day <strong>and</strong> as many as 800<br />
during her lifetime (usually about 300). The females are attracted <strong>by</strong> visual <strong>and</strong><br />
olfactory cues <strong>and</strong> normally choose the same kind of fruit during each oviposition<br />
cycle. Females usually die soon after they stop laying eggs. When the eggs hatch,<br />
the larvae promptly begin feeding on the pulp of fruits <strong>and</strong> about 15 days at a mean<br />
temperature of 25°C are necessary to complete their development.<br />
Figure 9. Ceratitis capitata adult female on a citrus fruit.<br />
Larvae pass through 3 instars. In cooler regions the species usually overwinters<br />
as pupa (while in warm climates it develops without interruptions), buried a few<br />
centimetres deep in the soil. In southern areas, a small number of individuals may<br />
also survive on late-season oranges. The pupa does not survive if temperatures are<br />
lower than 2°C for a week.<br />
Development of this fruit fly is mainly dependant on temperature. The optimum is<br />
around 32°C, which allows a generation to be completed in 2 weeks. Females will not<br />
oviposit when temperatures drop below 16°C, except when exposed to sunlight for
CITRUS PEST MANAGEMENT IN ITALY<br />
91<br />
several hours. Development stops at 10°C. Pupae carry the species through<br />
unfavourable conditions. During warm weather eggs hatch in 1.5–3 days. The duration<br />
of the egg stage is considerably increased <strong>by</strong> lower temperatures. Larval life may be as<br />
short as 6–10 days when the mean temperatures average 25-26.1°C. The kind <strong>and</strong><br />
ripening conditions of the fruit often influence the length of the larval stage. In citrus<br />
fruits, especially limes <strong>and</strong> lemons, it appears to be longer. Thus, larvae require 14–26<br />
days to reach maturity in a ripe lemon, as compared with 10–15 days in a green peach.<br />
Mature larvae, which are able to jump, leave the fruit in largest numbers at or just after<br />
daybreak <strong>and</strong> pupate in soil. Minimum duration of the pupal stage is 6–13 days when<br />
the mean temperature ranges from about 24.4 to 26.1°C.<br />
The largest numbers of adults emerge early in the morning during warm weather<br />
<strong>and</strong> more sporadically during cool weather. They can actively fly short distances,<br />
although they can cover longer distances carried <strong>by</strong> the wind. Newly emerged adults<br />
are not sexually mature. Males often show sexual activity 4 days after emergence.<br />
They produce a sexual pheromone which attracts females but is also perceived <strong>by</strong><br />
other males <strong>and</strong> even <strong>by</strong> human olfaction. Both sexes are sexually active throughout<br />
the day. When the daily mean temperature averages 24.4–25.6°C most females are<br />
ready to mate from 6 to 8 days after eclosion. Mating lasts from 2 to 4 h; males<br />
usually mate several times, while 60% of females mate only once.<br />
The Mediterranean fruit fly is one most noxious fruit pests in the world. Because<br />
of its worldwide distribution, its ability to tolerate colder climates better than most<br />
other species of fruit flies, <strong>and</strong> its wide range of hosts, it is ranked first among<br />
economically important fruit fly species. In some of the Mediterranean countries,<br />
only the earlier varieties of citrus are grown, because the flies develop so rapidly<br />
that late season fruits are too heavily infested to be marketable. Harvesting before<br />
complete maturity also is practiced in Mediterranean areas generally infested with<br />
this fruit fly.<br />
The damage caused <strong>by</strong> C. capitata is considerable, particularly in summer <strong>and</strong><br />
autumn. Infestation is indicated on the fruit <strong>by</strong> a variously coloured area, depending<br />
on the host, surrounding the oviposition puncture. Rotting of the underlying tissue<br />
causes a depression on the surface <strong>and</strong> the fruit drops prematurely. Even if a fruit<br />
has only been pierced for egg laying (without actual presence of living instars), it is<br />
totally unsaleable. On citrus fruits the oviposition punctures cause acceleration in the<br />
ripening process of the external tissues <strong>and</strong> the subsequent early drop of the fruits,<br />
also because of the occurrence of secondary infestations <strong>and</strong> infections.<br />
The constant global exchanges of goods <strong>and</strong> people may greatly facilitate<br />
transportation of the Mediterranean fruit fly in areas where it is not yet present,<br />
therefore making the efforts to contain it within its current distribution almost<br />
useless. Once the species is established, eradication efforts may be extremely<br />
difficult <strong>and</strong> expensive. In addition to reduction of crop yield, infested areas have<br />
the additional expense of control measures <strong>and</strong> costly sorting processes for both<br />
fresh <strong>and</strong> processed fruit <strong>and</strong> vegetables. Besides, the presence of C. capitata may<br />
strongly affect exportation to those countries where the species is not present or<br />
permanently established.<br />
Several species of entomophagous have been reported in the entire area of<br />
distribution of this fruit fly. Some of them have been imported from Africa <strong>and</strong>
92<br />
L. ZAPPALÀ<br />
Australia. Effective parasitoids of C. capitata are Psyttalia concolor (Szlep.)<br />
(Hymenoptera: Braconidae) <strong>and</strong> Pachyneuron vindemmiae (Rond.) (Hymenoptera:<br />
Pteromalidae). Efforts have been made to develop biological control programs using<br />
P. concolor, but with very limited success. This is mainly due to the high intrinsic<br />
rate of increase of the Mediterranean fruit fly <strong>and</strong> also to the behaviour of larvae,<br />
which feed <strong>and</strong> develop inside the fruits <strong>and</strong> therefore easily escape parasitization <strong>by</strong><br />
braconid wasps, especially when infesting large fruits. In the Mediterranean basin,<br />
natural control is mainly carried out <strong>by</strong> micro<strong>org</strong>anisms <strong>and</strong> occasional predators<br />
(Coleoptera Carabidae <strong>and</strong> Staphylinidae, Hymenoptera Formicidae of the genus<br />
Crematogaster), mostly active in soil against larvae <strong>and</strong> pupae.<br />
Cultural control methods, such as reducing the favourable host plants<br />
consociations, eliminating the infestation site <strong>and</strong> destroying infested fruits, are<br />
fundamental elements in field programs aiming at reducing the Mediterranean fruit<br />
fly populations.<br />
Chromotropic <strong>and</strong> chemotropic traps are used to attract adults. Males of C.<br />
capitata are known to be attracted <strong>by</strong> essential oils from Angelica archangelica L.,<br />
which contain several sesquiterpene hydrocarbons (α-copaene, α-ylangene, etc.).<br />
The same kind of molecules are also contained in cori<strong>and</strong>er, mint, thyme <strong>and</strong> citrus<br />
essence. However, none of these compounds found practical application, differently<br />
from what happened for esters of the methylcyclohexanecarboxylic acid: siglure,<br />
medlure, trimedlure. Other attractants commonly used are also ammonium<br />
compounds (diammonium phosphate) <strong>and</strong> hydrolyzed proteins. These compounds<br />
attract both males <strong>and</strong> females (while parapheromones attract only males) within a<br />
range of 20 m, but they mainly attract females looking for proteins. However these<br />
attractants are less selective towards beneficials.<br />
A possible control method is the “attract <strong>and</strong> kill” technique which is based on<br />
the use of devices pre-treated with a pyrethroid (mainly deltamethrin or lambdacyhalothrin)<br />
<strong>and</strong> activated with trimedlure or with hydrolyzed proteins. This<br />
technique is suggested on orchards with a minimum extension of 5 ha, unless they<br />
are isolated enough.<br />
Chemical control can be performed using deltamethrin, etofenprox, phosmet <strong>and</strong><br />
spinosad bait which has been recently authorized on citrus in <strong>Italy</strong>. In order to<br />
contain the negative secondary effects on the biocenosis it is highly recommended to<br />
perform localized treatments adding protein baits to the toxic compound. The<br />
treatments should be started in mid-July <strong>and</strong> repeated every 25–30 days, spraying<br />
trees only partially on one every two–three rows, <strong>and</strong> using around 200 l of solution<br />
per hectare. The treatments should be extended to the whole orchard when 20 or<br />
more adults are captured on the traps <strong>and</strong>/or after the first punctures on the fruits are<br />
observed. The results of trials carried out to evaluate in the field the repellent <strong>and</strong><br />
oviposition deterrent effect of clays <strong>and</strong> copper products, that can also be used in<br />
<strong>org</strong>anic groves, showed that kaolin can be applied to reduce the percentange of<br />
infested fruits (showing C. capitata punctures) at harvest (Caleca, Lo Verde,<br />
Palumbo Piccionello, & Rizzo, 2008).<br />
In several countries severe quarantine measures are applied, strongly affecting<br />
importation, in order to avoid the introduction <strong>and</strong> the permanent establishment of<br />
the Mediterranean fruit fly. Infested or potentially infested fruits are rejected or
CITRUS PEST MANAGEMENT IN ITALY<br />
93<br />
treated with fumigants or with low temperatures (2 weeks at 1°C), in order to<br />
eliminate all living instars present inside the fruits.<br />
3. SECONDARY PESTS<br />
Whiteflies, <strong>and</strong> namely the Woolly whitefly A. floccosus, are among the arthropod<br />
pests whose infestations in <strong>Italy</strong> greatly decreased over the last decades. Initially A.<br />
floccosus was considered of great economic importance because of the serious<br />
damage it can cause, mainly due to the very large amount of phloem sap sucked out<br />
from all parts of the tree both <strong>by</strong> the adults <strong>and</strong> the nymphs <strong>and</strong> the consequent<br />
production of huge amounts of honeydew. In case of strong infestations <strong>by</strong> this<br />
whitefly, blacken of citrus plants <strong>by</strong> sooty moulds is conspicuous <strong>and</strong> in such<br />
situations, honeydew, sooty mould <strong>and</strong> waxy secretions tend to mix up together,<br />
forming a continuous <strong>and</strong> hardly permeable cover on the lower surface of the leaves.<br />
Moreover, this whitefly has a strict relation with ants which protect the colonies<br />
interfering with the activity of natural enemies of this <strong>and</strong> also of other pests.<br />
However, biological methods have proved effective in controlling this species.<br />
In particular after the arrival of A. floccosus in <strong>Italy</strong> (in the 1970s), the parasitoid<br />
Cales noacki Howard (Hymenoptera: Aphelinidae) was introduced. This species,<br />
native to South America, had already been imported in France in the 1970s (Onillon<br />
& Onillon, 1972) <strong>and</strong> was then introduced in Southern <strong>Italy</strong> in 1980 (Liotta &<br />
Maniglia, 1983; Longo, 1985). The beneficial insect was reared on its natural host,<br />
feeding on citrus trees both in insectaries <strong>and</strong> in the field. From these “bank plants”<br />
branches bearing parasitized whitefly colonies were collected <strong>and</strong> used to spread out<br />
the parasitoid in the field, directly <strong>by</strong> farmers. The parasitoid showed an intense<br />
activity reaching levels of parasitization higher than 80%, <strong>and</strong> managed to<br />
permanently establish also feeding on other hosts. It did not require further<br />
inoculations, except in orchards submitted to several chemical treatments (Longo et<br />
al., 1994). In the citrus growing areas where the climatic conditions are not<br />
unfavourable to the parasitoid (it is mainly affected <strong>by</strong> high summer temperatures)<br />
<strong>and</strong> where integrated pest management is performed with rational use of pesticides,<br />
the Woolly whitefly is almost always kept under adequate control <strong>by</strong> the aphelinid,<br />
without requiring further specific control treatments.<br />
Together with C. noacki, another parasitoid, the platygastrid Amitus spiniferus<br />
(Bréthes) was introduced, reared <strong>and</strong> released following the same technique used for<br />
the aphelinid. Although this second entomophagous was at first only found in low<br />
numbers <strong>and</strong> immediately after the releases, it is now quite widespread in all citrus<br />
growing areas <strong>and</strong> contributes to the control of A. floccosus infestations. Chemical<br />
control is therefore normally not necessary against the Woolly whitefly, at least in<br />
areas where natural enemies are protected <strong>and</strong> their action is promoted.<br />
Similarly, two other exotic whitefly species, D. citri <strong>and</strong> P. myricae, have been<br />
successfully contained in the framework of classical biological control programs.<br />
The first species, native to India, was first recorded in <strong>Italy</strong> in 1965 <strong>and</strong> initially<br />
caused very heavy infestations. Presently it has almost disappeared, thanks to the<br />
effective control performed <strong>by</strong> the parasitoid Encarsia lahorensis (Howard)
94<br />
L. ZAPPALÀ<br />
(Hymenoptera: Aphelinidae) introduced in <strong>Italy</strong> from California in 1973 (Viggiani<br />
& Mazzone, 1978). The entomophagous was distributed throughout the main citrus<br />
growing areas of Southern <strong>Italy</strong> using plants or parts of plants bearing Citrus<br />
whitefly parasitized colonies. It permanently established <strong>and</strong> managed to effectively<br />
control the populations of the pest which rapidly became a species of minor<br />
importance in Italian citrus orchards (Longo et al., 1994).<br />
In 1990 the Japanese bayberry whitefly, P. myricae, was reported for the first<br />
time in <strong>Italy</strong> (Rapisarda, Siscaro, Leocata, & Asero, 1990). This polivoltine,<br />
polyphagous homopteran, with a strong tendency to parthenogenesis, is highly<br />
efficient in colonizing new areas. It mainly develops on new shoots <strong>and</strong> frequently<br />
lays eggs along the leaf margin which at maturity show a typical serrate aspect.<br />
Several parasitoids, such as the aphelinids C. noacki <strong>and</strong> Encarsia meritoria Gahan,<br />
adapted to develop on this whitefly without, however, successfully containing its<br />
populations. Therefore, in order to enlarge the parasitic complex, the aphelinid<br />
Eretmocerus debachi Rose & Rosen was imported from Israel in several citrus<br />
growing regions. The newly introduced entomophagous established, rapidly reached<br />
parasitization levels of 20–30% <strong>and</strong> showed a remarkable spreading capacity.<br />
Thanks to these characteristics the endoparasitoid managed to successfully control<br />
the whitefly as it had already happened in other Mediterranean citrus growing areas<br />
(Rose, De Bach, & Woolley, 1981). The Japanese bayberry whitefly is now only<br />
very rarely present in citrus orchards <strong>and</strong> no chemical treatment is required, because<br />
of the effective control performed <strong>by</strong> its natural enemies.<br />
Finally, other pests, which are normally considered as secondary since they are<br />
kept under control <strong>by</strong> a rational agronomic management of the orchard, <strong>by</strong> a reduced<br />
use of pesticides <strong>and</strong> <strong>by</strong> an effective natural enemies complex, are: the soft scales<br />
Ceroplastes rusci, Coccus hesperidum L. <strong>and</strong> Saissetia oleae, the armoured scale<br />
Parlatoria perg<strong>and</strong>ii, the moths Prays citri Mill. <strong>and</strong> Archips rosanus. Three species<br />
of aphids [Aphis spiraecola, A. gossypii <strong>and</strong> Toxoptera aurantii (B.d.F.)] are<br />
considered particularly noxious to young <strong>and</strong> regrafted trees. However, the direct<br />
damage caused <strong>by</strong> these pests is <strong>by</strong> far less important than the indirect damage<br />
related to their capacity of transmitting viral diseases <strong>and</strong> namely the Citrus Tristeza<br />
Virus. In particular A. gossypii is considered, in the Mediterranean basin as well as<br />
in other citrus growing regions of the world, the main vector of this virus in those<br />
areas where its most efficient specific aphid vector (Toxoptera citricidus) is still<br />
absent (Bar-Joseph & Loebenstein, 1973; Yokomi, Joost, & Backus, 2005).<br />
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Mineo, G., Mineo N., & Sinacori, A. (2001). Primi reperti sull’acclimatazione di Citrostichus<br />
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5<br />
ENTOMOPATHOGENIC NEMATODE ECOLOGY<br />
AND BIOLOGICAL CONTROL IN FLORIDA<br />
CITRUS ORCHARDS<br />
RAQUEL CAMPOS-HERRERA 1 , ROBIN J. STUART 1 , FAHIEM<br />
EL-BORAI 1, 2 , CARMEN GUTIERREZ 3 AND LARRY DUNCAN 1<br />
1 University of Florida, IFAS<br />
Citrus Research <strong>and</strong> Education Center,<br />
Lake Alfred, FL 33850, USA<br />
2 Plant Protection Department,<br />
Faculty of Agriculture,<br />
Zagazig University, Zagazig, Egypt<br />
3 Departamento de Agroecología, Instituto de Ciencias Agrarias,<br />
Centro de Ciencias Medioambientales CSIC,<br />
Madrid 28006, Spain<br />
Abstract. Biological control through augmentation of entomopathogenic nematodes (EPNs) in soil is an<br />
important component of integrated pest management (IPM) of the root weevil, Diaprepes abbreviatus, in<br />
Florida citrus orchards for over 20 years. However, to improve the effectiveness of EPNs for weevil<br />
control substantial information is needed about the post-application biology of EPNs as well as the<br />
ecology <strong>and</strong> importance of endemic species for weevil management. Current status of EPNs<br />
augmentation as a weevil control tactic, their role in soil food webs in different habitats, <strong>and</strong> the<br />
biocontrol potentials of endemic EPN communities, are reviewed. We also discuss molecular approaches<br />
to assess EPN population distribution <strong>and</strong> dynamics, <strong>and</strong> how these techniques could contribute to our<br />
underst<strong>and</strong>ing of nematodes ecology to enhance EPNs in biocontrol. Basic <strong>and</strong> applied study of EPNs<br />
increased during the past half-century, accelerating awareness of limitations for many conventional<br />
management practices. Underst<strong>and</strong>ing the EPNs population biology is necessary to discover <strong>and</strong> exploit<br />
new ways to increase their efficacy <strong>and</strong> reliability for biological control in managed ecosystems.<br />
1. INTRODUCTION<br />
Since the era of synthetic pesticide development accelerated in the mid-twentieth<br />
century, the management of citrus groves worldwide has generally evolved from a<br />
heavy reliance on prophylactic insecticide use to a more rational application of these<br />
101<br />
A. <strong>Ciancio</strong>, K.G. Mukerji (eds.), Integrated Management of Arthropod Pests<br />
<strong>and</strong> Insect Borne Diseases, Integrated Management of Plant Pests <strong>and</strong> Diseases 5,<br />
DOI 10.1007/978-90-481-8606-8_5, © Springer Science+Business Media B.V. 2010
102<br />
R. CAMPOS-HERRERA ET AL.<br />
chemicals within integrated pest management (IPM) programs. IPM typically<br />
reduces pesticide use <strong>by</strong> monitoring both pest <strong>and</strong> beneficial <strong>org</strong>anisms, <strong>and</strong><br />
predicting crop loss as the basis for management decisions (Timmer & Duncan,<br />
1999). Nevertheless, the quantities of synthetic pesticides used in orchards remain<br />
significant <strong>and</strong> pose serious threats to the environment, especially natural biological<br />
control processes, wildlife, groundwater contamination, resource depletion, <strong>and</strong><br />
human health <strong>and</strong> safety (Edwards, 1993; Pimentell et al., 1993). Recognition of<br />
these concerns has led to increased interest in <strong>org</strong>anic methods for crop <strong>and</strong> pest<br />
management in citriculture; <strong>and</strong> biological control, whether conducted as classical,<br />
augmentation or conservation biological control, necessarily plays a pivotal role.<br />
When considering the costs <strong>and</strong> benefits of various management paradigms, it is<br />
noteworthy that increased chemical inputs do not necessarily result in increased<br />
output per unit area. In the Mediterranean Basin, Spanish <strong>and</strong> Italian citrus growers<br />
use 4-fold <strong>and</strong> 15-fold greater quantities of pesticides than do Greek growers, but<br />
obtain similar citrus production per hectare (Gutiérrez et al., 2005). Nevertheless,<br />
pest management is of frequent <strong>and</strong> critical concern in all agricultural endeavours,<br />
<strong>and</strong> the development of sustainable pest management systems requires a<br />
fundamental underst<strong>and</strong>ing of how populations of pests <strong>and</strong> their natural enemies<br />
behave in specific crop habitats (Hoy & Herzog, 1985; Flint & Dreistadt, 1998;<br />
Rechcigl & Rechcigl, 2000; Horowitz & Ishaaya, 2004).<br />
In Florida citrus orchards, pesticide use during the last quarter of the twentieth<br />
century decreased steadily as a succession of pests were shown to be manageable<br />
through biological control <strong>by</strong> endemic or introduced natural enemies. Growers<br />
learned that fruit destined for juice processing could usually be produced without the<br />
use of insecticides <strong>and</strong> that fruit grown for the fresh market often required no more<br />
than a few well-timed pesticide treatments to manage mites <strong>and</strong> fungi that cause rind<br />
blemishes. Copper sprays <strong>and</strong> petroleum oils were the primary pesticides used<br />
during this period, <strong>and</strong> serious outbreaks of scale <strong>and</strong> other soft body pests were rare<br />
<strong>and</strong> almost always associated with disruption of biological control through<br />
unnecessary use of pesticides.<br />
Unfortunately, the limited use of pesticides <strong>and</strong> widespread success of<br />
biological control in Florida citrus groves came to an abrupt halt when the<br />
devastating bacterial disease known as “Huanglongbing” or “citrus greening” caused<br />
<strong>by</strong> the bacterium C<strong>and</strong>idatus Liberibacter asiaticus, was detected in the state for the<br />
first time in 2005. Citrus greening is vectored <strong>by</strong> the Asian Citrus Psyllid,<br />
Diaphorina citri, infects all known citrus cultivars, spreads rapidly, <strong>and</strong> is lethal to<br />
trees. Growers attempt to slow the spread of the disease <strong>by</strong> removing infected trees<br />
<strong>and</strong> suppressing the vector with frequent applications of systemic <strong>and</strong> topical<br />
insecticides. Consequently <strong>and</strong> predictably, many secondary pests are increasing in<br />
Florida citrus orchards, <strong>and</strong> psyllid resistance to most classes of insecticides is<br />
becoming widespread. Moreover, the increased production costs <strong>and</strong> diminishing<br />
effectiveness of these intensive pest management practices are coinciding with lower<br />
citrus prices, largely due to the increased availability of other fruit juices, to<br />
significantly lower the profitability of Florida citriculture. In view of this crisis, the<br />
future of the Florida citrus industry is uncertain. However, fundamental research to<br />
underst<strong>and</strong> <strong>and</strong> control citrus greening is being heavily supported <strong>by</strong> federal, state
IPM THROUGH ENTOMOPARASITES<br />
103<br />
<strong>and</strong> private sources, <strong>and</strong> hopefully will lead to new <strong>and</strong> more effective strategies to<br />
deal with this problem.<br />
Prior to the introduction of citrus greening <strong>and</strong> its psyllid vector into Florida,<br />
the Diaprepes Root Weevil, Diaprepes abbreviatus, was considered the most<br />
important insect pest of citrus, <strong>and</strong> it remains a serious problem (Graham, McCoy, &<br />
Rogers, 1996; Graham, Bright, & McCoy, 2003; Duncan, Shapiro, McCoy, &<br />
Graham, 1999; McCoy, 1999). Like citrus greening, the weevil can kill trees <strong>and</strong><br />
cause entire orchards to become non-profitable in just a few years (Fig. 1) but,<br />
fortunately unlike greening, the most severe devastation appears limited to certain<br />
areas <strong>and</strong> grove conditions. For nearly 20 years, biological control through the<br />
augmentation of entomopathogenic nematodes (EPNs) to citrus soils has been an<br />
important component of weevil IPM in Florida <strong>and</strong> it continues to be an effective<br />
strategy in many groves. Moreover, recent research to improve the effectiveness of<br />
EPNs for weevil control has revealed substantial information about their postapplication<br />
biology as well as the ecology <strong>and</strong> potential importance of endemic EPN<br />
species for weevil management. In this chapter, we review the current status of EPN<br />
augmentation as a weevil control tactic in Florida citrus groves, the role of EPNs in<br />
soil food webs of different habitats in Florida, <strong>and</strong> possibilities for better exploiting<br />
the biocontrol potential of endemic EPN communities.<br />
Figure 1. Twenty-four-year-old citrus trees in flatwoods soil exhibiting typical<br />
symptoms of Diaprepes/Phytophthora pest-disease complex.
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R. CAMPOS-HERRERA ET AL.<br />
2. IPM OF THE DIAPREPES-PHYTOPHTHORA COMPLEX<br />
2.1. Diaprepes Economic Importance, Biology <strong>and</strong> Management<br />
Diaprepes abbreviatus is highly polyphagous <strong>and</strong> a major economic pest not only of<br />
citrus, but of numerous ornamentals, vegetables, sugarcane, <strong>and</strong> other crops. It is<br />
native to the Caribbean where it has long been considered a serious agricultural pest<br />
(Wolcott, 1936). It was first detected in Florida in 1964 (Woodruff, 1964) <strong>and</strong> has<br />
spread to all citrus producing areas of the state. In 1997, the weevil was known to<br />
infest over 13,000 ha of commercial citrus <strong>and</strong> 50,,000 ha of other crops in 20<br />
Florida counties (Lapointe, Shapiro, & Bowman, 1999). Over the past 40 years,<br />
many citrus growers have experienced devastating losses of trees <strong>and</strong> entire groves<br />
due to D. abbreviatus. Annual losses <strong>and</strong> cost of control for the Diaprepes root<br />
weevil in Florida citrus were estimated at $72 million, whereas losses in<br />
ornamentals <strong>and</strong> vegetables were estimated at $2 million (Pena & Amalin, 2000).<br />
Diaprepes abbreviatus recently became established in Texas <strong>and</strong> California where it<br />
is considered a major threat to agriculture <strong>and</strong> is the subject of quarantine <strong>and</strong><br />
eradication programs.<br />
The life cycle of this weevil is marked <strong>by</strong> lack of synchrony <strong>and</strong> extensive<br />
variability, characteristics that make it particularly difficult to control (McCoy, 1999).<br />
In Florida, adult D. abbreviatus emerge from soil throughout the year with a<br />
significant peak in spring <strong>and</strong> sometimes autumn (Stansly, Mizell, & McCoy, 1997;<br />
Duncan, McCoy, Stansly, Graham, & Mizell, 2001). The adults feed on new foliage,<br />
mating occurs in the canopy, <strong>and</strong> eggs are laid in masses glued between leaves <strong>by</strong> the<br />
ovipositing female. Individual females can produce more than 20,000 eggs during a<br />
lifetime that can last almost a year. The larvae hatch, drop to the soil, <strong>and</strong> burrow<br />
down to the roots where they begin feeding. As they grow, the larvae feed on larger<br />
roots, <strong>and</strong> pupation occurs in the soil after 9–11 larval instars. Typically, a broad range<br />
of instars occur in the soil simultaneously (Woodruff, 1985; Quintela, Fan, & McCoy,<br />
1998; McCoy, 1999; McCoy, Stuart, & Nigg, 2003; Nigg et al., 2003).<br />
Diaprepes abbreviatus feeding damage to the roots of citrus trees can be<br />
extensive (Fig. 2). Major structural roots are often girdled <strong>and</strong> killed; <strong>and</strong>, if the<br />
crown is girdled, then the tree dies. However, tree damage is greatest in the presence<br />
of the plant pathogenic oomycetes Phytophthora nicotianae or P. palmivora, which<br />
invade the roots at weevil feeding sites. The pest-disease complex is particularly<br />
severe in poorly drained soils that favor infection <strong>by</strong> the fungal zoospores (Graham<br />
et al., 1996; Duncan et al., 1999; McCoy, 1999).<br />
Control measures for D. abbreviatus include chemical insecticides, which can<br />
be applied as adulticides, egg sterilants, or soil barrier treatments for neonates<br />
(McCoy et al., 2009). The efficacy of all treatments is short-lived; <strong>and</strong>, therefore, in<br />
order to kill the maximum number of insects, growers are advised to monitor adult<br />
weevils as they emerge from soil <strong>and</strong> occupy the tree canopy. Pesticides should be<br />
applied at the onset of egg-laying, approximately 10 days following peak adult<br />
emergence. Nevertheless, because of the non-synchronous life cycle of this weevil,<br />
pesticides must be applied repeatedly to be effective, <strong>and</strong> such repeated applications<br />
can disrupt natural enemies <strong>and</strong> lead to additional pest problems. Moreover, the
IPM THROUGH ENTOMOPARASITES<br />
105<br />
present chemical controls are only marginally effective compared to the<br />
<strong>org</strong>anochlorine soil pesticides that were used previously <strong>and</strong> are now banned for<br />
environmental reasons (Duncan et al., 1999; McCoy, 1999).<br />
At present, the only recommended control for D. abbreviatus larvae in soil is the<br />
application of EPNs twice per year (Bullock, Pelosi, & Kidler, 1999; Duncan & McCoy,<br />
1996; Duncan, McCoy, & Terranova, 1996, Duncan et al., 2007; McCoy, 1999; McCoy,<br />
Shapiro, Duncan, & Nguyen, 2000). In the absence of pesticides, EPN augmentation<br />
twice annually in orchards on coarse s<strong>and</strong>y soil was shown to reduce adult weevil<br />
populations <strong>by</strong> more than half (Duncan et al., 2003, 2007).<br />
Figure 2. Excavated root system of 3-year-old citrus tree heavily damaged <strong>by</strong><br />
Diaprepes abbreviatus larval feeding. Note the deep channels in major roots which<br />
provide infection courts for Phytophthora spp.<br />
2.2. EPN Biology <strong>and</strong> Use in IPM Programs<br />
Entomopathogenic nematodes in the genera Steinernema <strong>and</strong> Heterorhabditis are<br />
obligate lethal parasites of insects <strong>and</strong> are an attractive alternative to chemical<br />
insecticides because they kill insect pests very quickly, are safe to mammals, <strong>and</strong> have<br />
little or no direct effect on nontarget <strong>org</strong>anisms (Bathon, 1996; Ge<strong>org</strong>is, Kaya, &<br />
Gaugler, 1991). These nematodes typically occur in the soil <strong>and</strong> have an<br />
environmentally-resistant non-feeding infective juvenile (IJ) stage that actively seeks<br />
out <strong>and</strong> kills insect hosts (Kaya, 1990; Lewis, Gaugler, & Kaya, 1992; Grewal &<br />
Ge<strong>org</strong>is, 1998). The nematodes kill their hosts with the aid of symbiotic<br />
entomopathogenic bacteria in the genera Photorhabdus <strong>and</strong> Xenorhabdus for
106<br />
R. CAMPOS-HERRERA ET AL.<br />
Heterorhabditis <strong>and</strong> Steinernema, respectively. The bacteria are carried in the nematode<br />
intestine <strong>and</strong> released into the host upon infection (Poinar, 1990). Insect death usually<br />
occurs within 72 h of infection, <strong>and</strong> the nematodes feed, develop to adults, <strong>and</strong><br />
reproduce within the host, often completing 2–3 generations, before producing a new<br />
generation of specialized IJs, which emerge from the cadaver <strong>and</strong> seek new insect hosts<br />
(Poinar, 1990). Because of their established safety to non-target <strong>org</strong>anisms, EPNs are<br />
exempt from pesticide registration with the Environmental Protection Agency in the<br />
United States <strong>and</strong> are similarly exempt in many other countries.<br />
EPNs have been used effectively in classical biological control programs. For<br />
example, Steinernema scapterisci was discovered in Uruguay, near the presumed<br />
center of origin of the mole cricket (Scapteriscus spp.). The nematode was<br />
introduced into Florida where it is now established <strong>and</strong>, in combination with<br />
introduced parasitoids, provides effective biological control of several invasive mole<br />
cricket species (Nguyen & Smart, 1990; Adjei, Smart, Frank, & Leppla, 2006). Most<br />
commonly, however, EPNs are used for augmentation biological control where they<br />
function as biopesticides <strong>and</strong> treatment efficacy is expected to be of short duration,<br />
typically a matter of 1–2 weeks (McCoy et al., 2000; Duncan et al., 2003, 2007). In<br />
such programs, EPNs function in the same manner as non-persistent chemical<br />
pesticides <strong>and</strong> are applied repeatedly, as needed.<br />
Surveys have shown that some naturally occurring EPNs are more abundant in<br />
undisturbed compared to intensively farmed habitats (Campos-Herrera et al., 2008), <strong>and</strong><br />
that use of various animal manure mulches can increase the prevalence of some EPNs<br />
(Bednarek & Gaugler, 1997; Duncan et al., 2007). Such observations suggest the<br />
possibility of developing conservation biological control tactics <strong>by</strong> which agricultural or<br />
other managed habitats are modified in ways that enhance natural control of arthropods<br />
<strong>by</strong> EPNs. However, reliable <strong>and</strong> effective conservation biological control tactics are as<br />
yet unknown <strong>and</strong> remain a matter of speculation (Lewis, Campbell, & Gaugler, 1998;<br />
Stuart, Barbercheck, Grewal, Taylor, & Hoy, 2006).<br />
In the Florida citrus industry, Steinernema carpocapsae was the first nematode to<br />
be developed commercially for root weevil control (Schroeder, 1987; Figueroa &<br />
Roman, 1990; Smith, 1994) but a further discovered species, S. riobrave (formerly S.<br />
riobravis) (Cabanillas, Poinar, & Raulston, 1994), was found to cause greater D.<br />
abbreviatus mortality (Schroeder, 1994; Duncan et al., 1996; Bullock et al., 1999) with<br />
some field studies reporting ~90% suppression (Duncan & McCoy, 1996; Duncan et<br />
al., 1996; Bullock et al., 1999). However, estimates of the efficacy <strong>and</strong> profitability of<br />
using EPNs for weevil control in citrus vary widely <strong>and</strong> probably reflect variation in<br />
factors such as product quality, application rates, suitability of edaphic conditions for<br />
EPNs, <strong>and</strong> experimental methods (Adair, 1994; Duncan et al., 1996; Duncan, Graham,<br />
& Zellers, 2002; Duncan et al., 2003; 2007; Bullock et al., 1999; Stansly et al., 1997;<br />
McCoy et al., 2000; McCoy, Stuart, Duncan, & Nguyen, 2002). Currently, S. riobrave<br />
is marketed in Florida under the br<strong>and</strong> name Bio Vector 355 (Becker Underwood Inc.,<br />
Ames, IA) <strong>and</strong>, in 1999, approximately 19,000 ha of citrus were treated with this<br />
product to control citrus root weevils (Dimock, personal communication).<br />
Despite the evident <strong>and</strong> long-recognized potential of EPNs for insect pest<br />
management <strong>and</strong> the commercial development of effective EPN products for<br />
augmentation, their market penetration <strong>and</strong> incorporation into broadly applied IPM
IPM THROUGH ENTOMOPARASITES<br />
107<br />
programs has been disappointing. In some crop-pest systems for which EPNs<br />
appeared promising, use of chemical pesticides or transformation of crop cultivars to<br />
express Bacillus thuringiensis toxins provided cheaper management options (Lewis<br />
et al., 1998; Shapiro-Ilan, Gouge, & Koppenhöfer, 2002). However, the greatest<br />
impediment to the use of EPNs is that they often appear less reliable <strong>and</strong> less<br />
effective than available chemical pesticides (Lewis et al., 1998). Extreme variability<br />
of soil physical <strong>and</strong> biological properties, even at a small scale, is probably one of<br />
the major causes of inconsistent performance of EPNs <strong>and</strong> most other soilborne<br />
biological control agents. Indeed, it would be remarkable if a single <strong>org</strong>anism was<br />
able to provide consistently high pest control in the myriad soil habitats encountered<br />
in most crops. Moreover, although EPNs can be isolated from most soil habitats,<br />
EPN distributions are typically patchy <strong>and</strong> their equilibrium densities low, <strong>and</strong> these<br />
patterns tend to be quickly reestablished following an augmentation event (McCoy<br />
et al., 2000; Duncan et al., 2007). Habitats that support EPN equilibrium densities<br />
high enough <strong>and</strong> uniform enough to be suppressive to arthropod pests are apparently<br />
rare but, when identified, could reveal important traits <strong>and</strong> environmental conditions<br />
amenable to a conservation biocontrol approach involving EPNs. Advantages of<br />
such an approach could include an increase in the duration of EPN efficacy <strong>and</strong>,<br />
consequently, a reduction or elimination of the need for periodic augmentation of<br />
commercially formulated EPNs or use of chemical pesticides.<br />
2.3. Spatial Relationships Between Soils, Root Weevils <strong>and</strong> Endemic EPNs<br />
Damage to citrus caused <strong>by</strong> the Diaprepes root weevil is related to regional <strong>and</strong> local<br />
variation in orchard soils. Trees growing in finer textured soils or in low, wet areas are<br />
often more heavily damaged than trees growing in well drained, coarser textured soils.<br />
This undoubtedly is due at least in part to a higher incidence of Phytophthora spp. in<br />
finer, wetter soils. However, soil conditions also appear to have a large effect on<br />
weevil abundance. A 3-year survey of six orchards in which weevil abundance was<br />
measured weekly revealed a 10-fold greater weevil abundance in finer textured<br />
compared to coarser textured soils (Futch, Duncan, & Zekri, 2005). Florida citrus<br />
orchards are planted in regions characterized <strong>by</strong> different soil profiles. The “central<br />
ridge” is composed of very deep, well drained, uniformly s<strong>and</strong>y (>96% s<strong>and</strong>) soils. In<br />
contrast, the coastal <strong>and</strong> inl<strong>and</strong> “flatwoods” regions have greater variation in soil<br />
texture <strong>and</strong> shallow water tables that require tree rows to be planted on raised beds for<br />
drainage <strong>and</strong> adequate rooting volume. Many flatwoods soils are s<strong>and</strong>y (80–95%<br />
s<strong>and</strong>), but the particle sizes of the s<strong>and</strong> fractions are smaller on average than those that<br />
characterize soils on the central ridge. Thus, weevil-infested orchards on the central<br />
ridge often exhibit little damage <strong>by</strong> D. abbreviatus, whereas orchards on fine-textured,<br />
poorly drained flatwoods soils are sometimes ab<strong>and</strong>oned as unprofitable, due to an<br />
inability to manage the large weevil populations.<br />
Relationships between spatial patterns of D. abbreviatus <strong>and</strong> specific abiotic<br />
soil factors have been reported within <strong>and</strong> among sites (Li et al., 2003; Li,<br />
Syvertsen, McCoy, Stuart, & Schumann, 2004a; Li et al., 2007), but experimental<br />
evidence of direct causal relationships is lacking (Li et al., 2004b). Nonetheless, a<br />
growing body of evidence suggests that soils influence D. abbreviatus populations
108<br />
R. CAMPOS-HERRERA ET AL.<br />
indirectly <strong>by</strong> affecting the community composition <strong>and</strong> predatory efficacy of<br />
endemic EPN species. Surveys that measured numbers of Diaprepes larvae falling<br />
from the canopy to the soil <strong>and</strong> numbers of adult weevils emerging from the soil<br />
over the course of 2 years concluded that the net survival rate from hatched egg to<br />
teneral adult is ~ 0.7–1.6% (McCoy et al., 2003).<br />
Figure 3. Representation of EPN population density distribution using a biplot in which<br />
vectors show the loading factors of the original variables on the associated factorial axes.<br />
(a) Association with cultural practices: NA, natural area, OPC, <strong>org</strong>anic perennial crop, CPC,<br />
conventional perennial crop, OAC, <strong>org</strong>anic annual crop, CAC, conventional annual crop.<br />
(b) Association with s<strong>and</strong>, silt <strong>and</strong> clay contents, available water, <strong>and</strong> <strong>org</strong>anic N, Zn <strong>and</strong> Cu<br />
concentrations. Circles show EPN population density <strong>by</strong> increasing the diameter as<br />
population size increases (from Campos-Herrera et al., 2008).
IPM THROUGH ENTOMOPARASITES<br />
109<br />
Therefore, if EPNs are important weevil larva predators, relatively small<br />
reductions in the rate at which EPNs prey on weevils could have a<br />
disproportionately large effect on increasing the weevil survival rate <strong>and</strong>, hence, the<br />
numbers of egg-laying adults in an orchard. Duncan et al. (2003, 2007) found that<br />
caged weevil larvae buried in orchards on the central ridge are killed, primarily <strong>by</strong><br />
endemic EPNs, at an average rate of 53% per week (range 38–82%) compared to<br />
110<br />
R. CAMPOS-HERRERA ET AL.<br />
highest on the central ridge (2.4), with significantly fewer (1.7) in the central<br />
flatwoods. To date, H. indica is the only species that has been encountered in<br />
significant numbers in the coastal flatwoods. A propensity for H. indica to occupy<br />
coastal habitats also has been noted in other parts of the Caribbean Basin (Fisher-Le<br />
Saux, Mauléon, Constan, Brunel, & Boemare, 1998; Mauléon, Denon, Bri<strong>and</strong>, 2006).<br />
Little is known about the direct effects of soil physical <strong>and</strong> chemical properties<br />
on the population biology of the Diaprepes root weevil. However, the various<br />
findings reviewed above provide evidence for the hypothesis that patterns of D.<br />
abbreviatus within <strong>and</strong> among Florida citrus orchards are partly regulated <strong>by</strong> the<br />
ways in which soil properties affect the natural enemies of D. abbreviatus. More<br />
explicitly, they suggest that EPNs might help regulate D. abbreviatus on the central<br />
ridge to the extent that it is often a minor pest, whereas reduced EPN predation in<br />
some flatwoods orchards may permit D. abbreviatus populations to attain highly<br />
damaging levels. If the natural control of D. abbreviatus <strong>by</strong> endemic EPNs varies in<br />
different regions of Florida, then underst<strong>and</strong>ing how these habitats influence EPN<br />
diversity <strong>and</strong> efficacy could be especially worthwhile <strong>by</strong> indicating strategies for<br />
conservation biological control through the manipulation of habitats to enhance the<br />
biocontrol potential of EPNs.<br />
Table 1. The frequency (% of samples) <strong>and</strong> average dominance (population density<br />
as a percentage of all EPN in the sample) a of five entomopathogenic nematodes in<br />
citrus orchards, in three regions of Florida b .<br />
Species<br />
Steinernema<br />
diaprepesi<br />
Ridge Central Flatwoods Coastal Flatwoods<br />
F D F D F D<br />
100 36 57 29 0 0<br />
S. riobrave 0 0 5
IPM THROUGH ENTOMOPARASITES<br />
111<br />
relative importance of biological interactions <strong>and</strong> how they may vary in different<br />
habitats (Kaya & Koppenhöfer, 1996). The profound complexity <strong>and</strong> variety of soil<br />
food webs makes it unlikely that key interactions between EPNs <strong>and</strong> other<br />
<strong>org</strong>anisms can be identified through highly controlled experimentation. However,<br />
molecular methods that can be used to identify <strong>and</strong> quantify <strong>org</strong>anisms at different<br />
trophic levels in soil provide cost-effective opportunities to survey natural soil<br />
communities in space <strong>and</strong> time in order to detect relationships that can then be<br />
studied for causality under controlled conditions.<br />
3.1. Soil Food Webs <strong>and</strong> EPN Spatial <strong>and</strong> Temporal Patterns<br />
Augmentation of EPNs in soil increases populations above an equilibrium density in<br />
order to increase the natural level of biological control. However, natural enemies<br />
of EPNs respond rapidly to the imbalance, so that EPN numbers <strong>and</strong> levels of<br />
biological control rarely exceed background levels for more than a few weeks<br />
(McCoy et al., 2000; Duncan et al., 2003, 2007; El-Borai et al., 2007). Populations<br />
of nematophagous mites <strong>and</strong> collembola have been shown to grow in response to<br />
EPN augmentation (Ishibashi, Young, Nakashima, Abiru, & Haraguchi, 1987;<br />
Epsky, Walter, & Capinera, 1988; Forschler & Gardner, 1991), <strong>and</strong> survival of<br />
augmented EPNs was inversely related to the final abundance of mites <strong>and</strong><br />
collembola in field plots (Wilson & Gaugler, 2004). Jaffee <strong>and</strong> Strong (2005)<br />
showed that propagules of some species of nematophagous fungi (NF) increase <strong>by</strong> 2<br />
orders of magnitude in a localized response to the emergence of thous<strong>and</strong>s of EPN<br />
IJs from an insect cadaver. Indeed, the bottom-up trophic cascade that results in<br />
more predators following EPN augmentation can apparently be large enough to<br />
sometimes reduce EPN populations below background levels for a short period until<br />
equilibrium is reestablished (Duncan et al., 2003, 2007). El-Borai et al. (2007)<br />
demonstrated that trophic cascades are modulated <strong>by</strong> the species <strong>and</strong> amount of<br />
EPNs added to the soil.<br />
Duncan et al. (2007) showed that treatments that either increased or decreased the<br />
population densities of various NF in the field also affected EPNs. Composted animal<br />
manure mulch reduced the abundance of trapping NF while increasing the numbers of<br />
sentinel insect larvae infected <strong>by</strong> EPNs. As noted above, augmenting the EPN<br />
community temporarily increased trapping <strong>and</strong> endoparasitic NF, <strong>and</strong> population<br />
growth of NF was sometimes followed <strong>by</strong> decreased sentinel infection <strong>by</strong> EPNs<br />
compared to non-augmented plots. The effects of these treatments suggest that NF<br />
population dynamics may affect the temporal <strong>and</strong> spatial patterns of EPN activity.<br />
However, the large variety of NF <strong>and</strong> EPN species, each with different life strategies,<br />
means that interactions between NF <strong>and</strong> EPNs are likely to be very complex. For<br />
example, during eight consecutive monthly sampling events, the prevalence of<br />
trapping NF in citrus field plots was inversely related to numbers of sentinel weevils<br />
infected <strong>by</strong> S. diaprepesi but positively related to those infected <strong>by</strong> H. zeal<strong>and</strong>ica in<br />
the succeeding month (Duncan et al., 2007). They proposed that these fungi might<br />
favor H. zeal<strong>and</strong>ica <strong>by</strong> more effectively suppressing its S. diaprepesi competitors.<br />
Timper <strong>and</strong> Kaya (1989) demonstrated that the NF Hirsutella rhossiliensis killed<br />
steinernematids much more effectively than heterorhabditids, <strong>and</strong> showed that the
112<br />
R. CAMPOS-HERRERA ET AL.<br />
infection peg of fungal spores did not penetrate beyond the second stage cuticle that is<br />
retained as a protective sheath <strong>by</strong> IJ (3rd stage) heterorhabditids. Steinernematid IJs<br />
generally cast the second stage cuticle shortly after emerging into the soil from insect<br />
cadavers (Timper & Kaya, 1989, 1992).<br />
A variety of mechanisms other than protective sheaths modulate predation <strong>by</strong><br />
NF on nematodes. For example, fungi that form adhesive networks trap plantparasitic<br />
root-knot nematodes much more effectively than cyst nematodes (neither of<br />
which retain a cast cuticle), whereas fungi producing constricting rings trapped both<br />
types of nematodes with equal efficiency (Jaffee, 1998). El-Borai et al. (2007)<br />
showed that in s<strong>and</strong> microcosms the predation rates of five species of endoparasitic<br />
<strong>and</strong> trapping NF on 5 EPN species, all commonly isolated from citrus orchards,<br />
were highly species specific. Two endoparasitic NF species that infect via zoospores<br />
were highly lethal to all EPN species except H. indica, which was unaffected <strong>by</strong><br />
these fungi in the microcosm assays. Conversely, large endemic steinernematids<br />
such as S. diaprepesi <strong>and</strong> Steinernema sp. (previously identified as S. glaseri) were<br />
relatively unaffected <strong>by</strong> several species of Arthrobotrys (trapping NF), compared to<br />
significant predation <strong>by</strong> these fungi on the smaller exotic S. riobrave <strong>and</strong> the<br />
heterorhabditids H. zeal<strong>and</strong>ica <strong>and</strong> H. indica. Thus, the report <strong>by</strong> El-Borai et al.<br />
(2007) did not support causality of the relationships between NF <strong>and</strong> S. diaprepesi<br />
or H. zeal<strong>and</strong>ica reported <strong>by</strong> Duncan et al. (2007). The lack of predation <strong>by</strong><br />
zoosporous NF on just H. indica is intriguing, however, since these commonly<br />
encountered NF require free water for zoospore movement <strong>and</strong> H. indica was the<br />
sole EPN species reported from several low lying coastal areas, which tend to have<br />
relatively wet soils (Fisher-Le Saux et al., 1998; Mauléon et al., 2006; Table 1).<br />
Organisms other than predators <strong>and</strong> parasites might influence the abundance of<br />
EPNs. Paenibacillus is a bacterial genus that is intimately associated with<br />
arthropods. Phoretic associations between Paenibacillus <strong>and</strong> EPNs were recently<br />
reported <strong>and</strong> demonstrate remarkable convergence of bacterial species adapting to<br />
two paraphyletic nematode genera (Enright & Griffin, 2004, 2005; El-Borai,<br />
Duncan, & Preston, 2005). Paenibacillus spp. associated with heterorhabditids have<br />
spindle shaped spores that adhere exclusively to the nematode sheath (2nd-stage<br />
cuticle) whereas those associated with steinernematids have oval spores that adhere<br />
only to the 3rd-stage cuticle (Fig. 4). Paenibacillus nematophilus spores attached to<br />
all tested heterorhabditid species <strong>and</strong> those in the closely-related order Stongylida<br />
(Enright & Griffin, 2004). In contrast, a Paenibacillus sp. associated with S.<br />
diaprepesi appears to be species specific (El-Borai et al., 2005). Paenibacillus spp.<br />
are frequently observed on all known endemic species of EPNs in Florida but not on<br />
the introduced species S. riobrave. Like the entomopathogenic bacteria P. popilliae<br />
<strong>and</strong> P. lentimorbus, the Paenibacillus species that are phoretic on EPN complete<br />
their life cycle in the insect cadaver but they are not entomopathogenic <strong>and</strong> they do<br />
not appear to affect the reproduction of EPN species. The only known adverse affect<br />
to the nematode is impaired motility in proportion to the degree to which a nematode<br />
is encumbered with spores. Spore-free steinernematids <strong>and</strong> heterorhabditids move<br />
further <strong>and</strong> infect more insects that do spore-encumbered nematodes. However, the<br />
degree to which Paenibacillus spp. can modulate EPN abundance in nature is<br />
unknown.
IPM THROUGH ENTOMOPARASITES<br />
113<br />
In addition, some opportunistic, free living nematodes are capable of entering<br />
insect cadavers <strong>and</strong> appropriating the nutients produced <strong>by</strong> the EPN-bacteria<br />
symbiosis to the extent that the EPNs fail to reproduce (Duncan et al., 2003; 2007).<br />
Some species of EPNs appear to be especially susceptible to this competitive<br />
displacement <strong>by</strong> free living species but, again, the significance of these interactions<br />
on EPN population dynamics is unknown. Clearly, much remains to be done to<br />
underst<strong>and</strong> how food web components interact to affect EPN patterns in space <strong>and</strong><br />
time.<br />
Figure 4. Cuticle of Steinernema diaprepesi heavily encumbered <strong>by</strong> spores of<br />
Paenibacillus sp., a non-pathogenic bacterium that reproduces within insects killed <strong>by</strong><br />
the nematode <strong>and</strong> its entomopathogenic symbiont, Xenorhabdus doucetiae. Movement<br />
through soil <strong>by</strong> infective juvenile nematodes is impeded <strong>by</strong> heavy infestations of<br />
Paenibacillus sp. Scale bar: 10 µm.<br />
3.2. Identifying Factors that Regulate EPN Abundance <strong>and</strong> Efficacy<br />
As noted previously, spatial surveys have revealed numerous relationships between<br />
EPN prevalence <strong>and</strong> various soil physical properties such as porosity (texture), water<br />
potential, chemistry, as well as cropping <strong>and</strong> management history. If causality can be<br />
demonstrated then some of these relationships have the potential to be exploited to<br />
develop cultural practices that enhance biological control. For example, some types of<br />
soil mulches have significantly enhanced populations of EPNs (Bednarek & Gaugler,<br />
1997; Duncan et al., 2007) whereas others appear to have no or negative effects on<br />
EPNs (Lacey, Arthurs, Unruh, Headrick, & Fritts, 2006). Bednarek <strong>and</strong> Gaugler
114<br />
R. CAMPOS-HERRERA ET AL.<br />
(1997) noted the apparent usefulness of composted animal manure for conservation<br />
biocontrol after showing that long-term applications of manure increased EPNs <strong>by</strong><br />
3-fold. Animal manure mulches likely increase availability of insect prey <strong>and</strong> were<br />
also shown to decrease the prevalence of some nematophagous fungi that prey on<br />
EPNs (Jaffee, Ferris, Stapleton, Norton, & Muldoon, 1994; Duncan et al., 2007). If a<br />
number of physical properties can be identified that consistently affect EPN spatial<br />
patterns then this information might be used to incrementally improve biological<br />
control achieved <strong>by</strong> either augmented or endemic EPNs.<br />
Underst<strong>and</strong>ing the basis of relationships between EPNs <strong>and</strong> other variables in<br />
the field can require a substantial research investment. Whereas EPN associations<br />
with some variables have a causative basis, others arise indirectly through the effects<br />
of unmeasured hidden variables. Therefore, identifying those variables that are most<br />
likely to modulate EPN prevalence or behavior in predictable ways is important. A<br />
comparison of the results of surveys using different sample criteria can be helpful in<br />
selecting variables of interest.<br />
Campos-Herrera et al. (2007) found that soil moisture was positively associated<br />
with EPN recovery frequency in a survey of 100 undisturbed sites (natural areas <strong>and</strong><br />
field borders) in La Rioja, Spain. However, in a temporal survey of 18 agricultural<br />
fields with different management regimes <strong>and</strong> bordering natural areas, EPNs were<br />
unrelated to soil moisture but inversely related to soil disturbance (Campos-Herrera et<br />
al., 2008). Because greater irrigation was employed in tilled annual cropping systems<br />
with few EPNs than in natural areas or <strong>org</strong>anically grown perennial crops with<br />
numerous EPNs, Campos Herrera et al. (2008) speculated that soil disturbance is more<br />
important than moisture in regulating EPN spatial patterns. Similarly, Campos-Herrera<br />
et al. (2008) reported linear correlations between EPNs <strong>and</strong> certain soil characteristics<br />
that were also studied <strong>by</strong> Alumai, Grewal, Hoy, <strong>and</strong> Willough<strong>by</strong>, (2006) <strong>and</strong> Duncan<br />
et al. (unpublished). Differences in the survey protocols among these studies suggest<br />
the possibility that some of the correlations between soil properties <strong>and</strong> EPNs are due<br />
to the influence of soil texture on both EPNs <strong>and</strong> certain chemical properties (Fig. 5).<br />
Because greater s<strong>and</strong> content of soil generally favors EPNs, chemical properties<br />
associated in some manner with s<strong>and</strong> content would likely be similarly associated with<br />
EPNs. The relationships measured in Ohio <strong>and</strong> Florida (shown in small font in Fig. 5)<br />
are strikingly similar. Organic matter, K + <strong>and</strong> Mg ++ tended to be negatively associated<br />
with both EPNs <strong>and</strong> percentage s<strong>and</strong> whereas P was positively associated with both<br />
variables. In contrast, these relationships had exactly opposite trends in the Spanish<br />
survey. Nevertheless, soil chemicals in each of the three surveys were associated with<br />
EPNs in the same manner that they were associated with percentage s<strong>and</strong>. The Ohio<br />
<strong>and</strong> Florida surveys occurred on several golf courses <strong>and</strong> within a single citrus<br />
orchard, respectively. Thus, cultural practices were similar among sites within each of<br />
these surveys, <strong>and</strong> the effects of porosity <strong>and</strong> soil colloid surfaces on leaching of some<br />
chemicals <strong>and</strong> the adsorption of others operated on similar levels of nutrient inputs.<br />
However, the Spanish survey compared EPN populations in natural areas <strong>and</strong> in a<br />
variety of different annual <strong>and</strong> perennial cropping systems. The very different levels of<br />
inputs between the Spanish sample sites might have caused different relationships<br />
between chemicals <strong>and</strong> percentage s<strong>and</strong> <strong>and</strong>, therefore, with EPNs than seen in Ohio<br />
or Florida.
IPM THROUGH ENTOMOPARASITES<br />
115<br />
Figure 5. Linear correlations relating soil chemical properties to either the numbers<br />
of entomopathogenic nematodes or percentage of s<strong>and</strong>, in samples taken to study EPN<br />
spatial patterns. Symbols in large font proceed from a survey of different cropping<br />
systems in La Rioja, Spain; remaining symbols derived from golf courses in Ohio <strong>and</strong><br />
a citrus orchard in Florida. Asterisks on the left side of symbols show correlation<br />
significance (*, P
116<br />
R. CAMPOS-HERRERA ET AL.<br />
endoparasitic fungi are obligate parasites of nematodes <strong>and</strong> some other microscopic<br />
metazoans (Kerry & Jaffee, 1997).<br />
Because the predation rate on EPNs cannot be reliably inferred from the<br />
abundance of many NF species in soil, more direct methods of assessing predation<br />
are needed. Duncan et al. (2007) developed an assay to enumerate NF species<br />
recovered directly from nematodes rather than soil, which better reflects levels of<br />
predatory rather than saprophytic behavior. Circumscribed soil cylinders were<br />
defined <strong>and</strong> isolated in situ <strong>by</strong> pounding PVC tubes to a depth of 20 cm in soil<br />
beneath the citrus tree canopy. These relatively undisturbed soil cylinders were<br />
baited with large numbers of EPNs <strong>and</strong> then recovered from the field after 3 days.<br />
The nematodes extracted from the soil cylinders were placed on water agar to allow<br />
growth of NF from nematode cadavers. This method effectively recovered predators<br />
<strong>and</strong> parasites of nematodes, which were invariably all killed within 5 days.<br />
However it was necessary to add fresh EPNs to the agar plates after 5 days to induce<br />
the formation of fungal fruiting bodies for species identification <strong>and</strong> the estimation<br />
of population abundance based on numbers of EPNs killed. The long period of time<br />
during which the fungi competed with one another on the water agar likely skewed<br />
the abundance estimates in favor of species best adapted to this artificial habitat.<br />
A more reliable estimate of NF predation rates in soil requires the identification<br />
of infected nematodes immediately following extraction from soil. Indeed, direct<br />
quantification of target populations rather than estimation from bioassays would<br />
facilitate underst<strong>and</strong>ing the roles in food webs of many <strong>org</strong>anisms that are currently<br />
poorly understood. For example, possible effects of Paenibacillus on EPN<br />
prevalence can be inferred in bioassays <strong>by</strong> the degree of spore encumbrance of EPN<br />
IJs emerging from sentinel insects (Duncan et al., 2007). However, spore<br />
encumbrance increases with the length of time that IJs are in the vicinity of bacteriainfected<br />
cadavers in these assays, <strong>and</strong> the detection of bacteria using sentinel insects<br />
depends on EPN abundance in soil. Therefore, methods to directly measure the<br />
abundance of these bacteria in soil or on nematodes extracted from soil are needed<br />
to accurately assess the degree to which EPNs <strong>and</strong> Paenibacillus interact at different<br />
times or in different habitats.<br />
Real-time PCR (or quantitative PCR, qPCR) provides an efficient method of<br />
quantifying soilborne <strong>org</strong>anisms such as bacteria <strong>and</strong> fungi using molecular probes<br />
(Atkins, Clark, P<strong>and</strong>e, Hirsch, & Kerry, 2005; Klob, Knief, Stubner, & Conrad,<br />
2003). The abundance of S. kraussei <strong>and</strong> S. affine in fields <strong>and</strong> meadows was<br />
recently compared using qPCR (Torr, Spiridonov, Heritage, & Wilson, 2007). The<br />
methods most commonly employed involve the use of fluorescent products that link<br />
to double str<strong>and</strong>ed DNA causing increased fluorescence (e.g., SYBR Green®) or the<br />
design of specific fluorescent probes (e.g., TaqMan® or hydrolysis probes). In both<br />
cases, species-specific primers designed for the target taxon are used. Both systems<br />
can function with a high degree of species specificity but, due to the use of a probe<br />
that adds an additional level of specificity to the primers, hydolysis probes are<br />
generally reported to be more reliable in this regard (Holeva et al., 2006; Leal,<br />
Green, Allen, Humble, & Rott, 2007). In both systems, the amount of fluorescence<br />
increases during PCR cycling. The quantification cycle (Cq) (also called threshold<br />
cycle or Ct) is that at which product amplification enters an exponential phase.
IPM THROUGH ENTOMOPARASITES<br />
117<br />
St<strong>and</strong>ard curves of Cq values from known quantities (e.g., numbers of <strong>org</strong>anisms or<br />
amounts of DNA) of the species in question can be developed in order to estimate<br />
quantities in unknown samples (Fig. 6). Developing the molecular components for a<br />
new target species requires several steps, each involving options that affect the cost,<br />
accuracy, or reliability of the final method (Fig. 7).<br />
Figure 6. Amplification curves for a qPCR assay with Steinernema diaprepesi as target<br />
species. Fluorescence intensities (a) produced <strong>by</strong> different nematode concentrations<br />
(1–300 infective juveniles) are shown <strong>by</strong> the different curves entering the exponential<br />
growth at different points (Cq) in the cycling series (NCT = negative control). Linear<br />
st<strong>and</strong>ard curve of the quantification cycle number (Cq) for the corresponding<br />
nematode numbers, expressed as log (b). All reactions performed in triplicate.<br />
The relatively few reports using qPCR to identify <strong>and</strong> quantify cryptic soilborne<br />
<strong>org</strong>anisms vary in the adequacy with which experiments are described in order to<br />
reproduce the work. Bustin et al. (2009) provide useful guidelines for the accurate
118<br />
R. CAMPOS-HERRERA ET AL.<br />
presentation of the methods <strong>and</strong> results obtained using qPCR. Some of methods<br />
reported to date are reviewed <strong>and</strong> compared.<br />
Most species-specific primers (<strong>and</strong> probes, if required) have been developed to<br />
amplify sections of the ITS region. This region of ribosomal DNA is usually well<br />
conserved at the species level but provides greater variability between species than<br />
more highly conserved regions such as D2–D3. Extensive interspecific variation is<br />
necessary to provide enough species-specific primer targets to identify those that<br />
will amplify segments of an optimum size for reliable qPCR reactions (i.e., between<br />
80 <strong>and</strong> 200 base pairs). Compared to other gene regions, the large ITS database in<br />
GenBank facilitates validating the species-specificity of ITS primers among<br />
<strong>org</strong>anisms characterized to date. In addition to ITS, other regions used to develop<br />
primers/probes for use in qPCR include 18S from rDNA (Holeva et al., 2006;<br />
MacMillan, Blok, Young, Crawford, & Wilson, 2006), MspI satDNA monomeric<br />
unit (François et al., 2007), Hsp70 sequence (Leal et al., 2007) <strong>and</strong> the intragenic<br />
spacer (IGS) region of the 5S rRNA gene (Kang, Moon, Lee, Shin, & Lee, 2009).<br />
Figure 7. General protocol to develop real time qPCR primers <strong>and</strong> probes (from<br />
Campos-Herrera, Johnson, El-Borai, Graham, Duncan, 2009).
IPM THROUGH ENTOMOPARASITES<br />
119<br />
Once the primers/probes have been validated, sampling <strong>and</strong> extraction methods<br />
can be selected that exploit the advantages <strong>and</strong> limitations of qPCR. Many protocols<br />
for sampling fungi <strong>and</strong> bacteria in soil extract DNA directly from soil samples that<br />
can be as small as a few grams or less. Smith <strong>and</strong> Jaffee (2009) suggest using a<br />
combination of culturing <strong>and</strong> molecular detection of trapping fungi because primers<br />
specific for a major group of trapping fungi (Orbiliales) yielded clones representing<br />
just 3 of 8 species that were isolated through culturing, but revealed the presence of<br />
18 species that had not been detected through culturing. It is unclear whether uneven<br />
distribution of the species in the small samples (12.5 cm 3 soil) affected the results.<br />
In order to optimize sampling <strong>and</strong> extraction methods, additional studies comparing<br />
both species-specific primers <strong>and</strong> culturing are needed, <strong>and</strong> they should involve<br />
DNA that has been extracted <strong>and</strong> concentrated from a range of soil sample sizes.<br />
MacMillan et al. (2006) accurately quantified numbers of slug-parasitic<br />
nematodes <strong>by</strong> extracting DNA directly from 10 g soil samples but were not able to<br />
do so from 1 g soil samples. However, the samples were artificially infested with<br />
nematodes <strong>and</strong>, in contrast to bacteria or fungal propagules, it is unlikely that the<br />
relatively low numbers of nematodes that occur naturally in soil can be reliably<br />
detected from such small samples. Studies <strong>and</strong> diagnostic services that use qPCR to<br />
quantify metazoans such as nematodes in soil routinely employ st<strong>and</strong>ard methods of<br />
sampling <strong>and</strong> extraction <strong>and</strong>, therefore, are able to rely on conventional sampling<br />
programs designed to optimize cost <strong>and</strong> accuracy (Hollaway, Ophel-Keller, Taylor,<br />
Burns, & McKay, 2004; Stirling et al., 2004; Ophel-Keller, McKay, Hartley,<br />
Herdina, & Curran, 2008; Donn, Griffiths, Nielson, & Daniell, 2008). Such<br />
programs employ a variety of sampling methods that address the highly aggregated<br />
spatial patterns of nematodes, usually <strong>by</strong> collecting large numbers of samples that<br />
are pooled, mixed <strong>and</strong> subsampled for nematode extraction (Been & Schomaker,<br />
2006).<br />
Subsamples of 500–1000 cm 3 are routinely processed <strong>by</strong> methods such as<br />
sucrose centrifugation to recover nematodes (Jenkins, 1964). There is no reason that<br />
such large subsamples cannot be used for molecular diagnostics although a number<br />
of studies report the use of smaller subsamples (Table 2), perhaps to reduce the<br />
recovery of soil chemicals that can interfere with DNA extraction <strong>and</strong> PCR reactions<br />
(see below). If the objective is estimating predation rates <strong>by</strong> measuring only those<br />
NF intimately associated with nematodes, the nematodes can be further separated<br />
from the small residue of soil remaining after sucrose centrifugation <strong>by</strong> additional<br />
centrifugation in a magnesium sulphate density gradient (Duncan et al., 2007).<br />
Preliminary experiments (Duncan et al., unpublished data) revealed less fungal DNA<br />
<strong>and</strong> fewer nematodes recovered following the two-step extraction procedure<br />
compared to just sucrose centrifugation; <strong>and</strong> there was no evidence of significant NF<br />
DNA in the soil residue. This observation should be confirmed using a variety of<br />
soils <strong>and</strong> NF targets because use of one rather than two extractions reduces time <strong>and</strong><br />
cost, <strong>and</strong> the recovery of more nematodes increases the detection efficiency of the<br />
system.<br />
A variety of methods have been used to extract nematode DNA from soil or<br />
from nematodes recovered from soil (Table 2). Kits involve higher costs than<br />
st<strong>and</strong>ard laboratory protocols to purify DNA but are far simpler <strong>and</strong> faster to use if
120<br />
R. CAMPOS-HERRERA ET AL.<br />
they perform well with material extracted from soil. When DNA was isolated<br />
directly from soil, the PowerMax Soil TM DNA Isolation Kit (MoBio) was more<br />
reliable than a st<strong>and</strong>ard laboratory method or the Ultra Clean Soil TM DNA Kit<br />
(MacMillan et al., 2006). For nematodes extracted from soil, Madami, Subbotin, <strong>and</strong><br />
Moens, (2005) concluded that the use of proteinase K followed <strong>by</strong> PCR Buffer<br />
yielded more DNA than if it was followed <strong>by</strong> Worm Lysis Buffer. Donn et al.<br />
(2008) found that use of sodium hydroxide extraction, ChargesSwitch PCR CleanUp<br />
Kit (Invitrogen), QIAquick PCR Purification System (Invitrogen) <strong>and</strong> the Wizard<br />
PCR Prep DNA Purification System (Promega) all failed to provide either enough<br />
DNA or DNA of high enough quality for PCR whereas phenol chloroform<br />
extraction or Purelink PCR Purification Columns (Invitrogen) provided high<br />
concentrations of DNA acceptable for PCR studies. Campos-Herrera et al. (2009)<br />
obtained good quality DNA from nematodes extracted with sucrose-centrifugation<br />
using the Unltra Clean Soil TM DNA Kit (Mo Bio).<br />
PCR can be inhibited <strong>by</strong> chemical contaminants in soil (e.g., humic acid,<br />
phenolic compounds) or <strong>by</strong> use of excessive template. Inhibition can be complete or<br />
partial, <strong>and</strong> so it is important to calibrate qPCR with results obtained from known<br />
quantities of the target <strong>org</strong>anism (e.g., nematodes, nematodes infected <strong>by</strong> NF, etc.)<br />
added to populations of nematodes extracted from soil rather than relying on PCR of<br />
DNA from pure cultures. Bovine serum albumin has been used to reduce the effects<br />
of chemical inhibitors of PCR (MacMillan et al., 2006; Torr et al., 2007; Campos-<br />
Herrera et al., 2009). To avoid excess template, dilution of DNA from 4 to 100-fold<br />
from samples of unknowns is usually necessary (Madami et al., 2005; Jones, Todd,<br />
& Herman, 2006; Kang et al., 2009). Because each soil sample yields a different<br />
quantity of DNA that might affect the reaction, the use of a st<strong>and</strong>ard DNA quantity<br />
is preferable to a st<strong>and</strong>ard dilution.<br />
Most authors report very high detection efficiency from the use of qPCR, which<br />
is frequently at the level of a single nematode. Several multiplex systems in which<br />
single reactions measure more than one nematode species or combinations of<br />
nematodes <strong>and</strong> fungi have been developed that can substantially reduce time <strong>and</strong><br />
cost (Madami, Ward, & de Boer, 2008; Jones et al., 2006; Berry, Fargette, Spaull,<br />
Mor<strong>and</strong>, & Cadet, 2008; Zijlstra & van Hoof, 2006). Unfortunately, the increased<br />
likelihood of competition between target DNA or development of interacting<br />
primers (primer-dimers) that increase florescence for a false signal can impede the<br />
development <strong>and</strong> performance of multiplex systems. Zijlstra <strong>and</strong> van Hoof (2006)<br />
reported a density-dependent reduction in the efficiency of multiplex qPCR <strong>and</strong><br />
suggested that individual reactions would be required for precise estimation. Berry<br />
et al. (2008) observed similarity of melting temperatures <strong>and</strong> competition between<br />
the amplification of Meloidogyne javanica <strong>and</strong> Pratylenchus zeae targets, which<br />
made it impossible to distinguish the two species in a multiplex reaction.<br />
At present, studies using molecular techniques to assess EPN population<br />
distribution <strong>and</strong> dynamics remain rare but the development <strong>and</strong> optimization of<br />
these techniques could contribute much to our underst<strong>and</strong>ing of these nematodes <strong>and</strong><br />
the kinds of strategies that might facilitate their enhanced usefulness for biological<br />
control in agroecosystems.
IPM THROUGH ENTOMOPARASITES 121
122<br />
R. CAMPOS-HERRERA ET AL.
IPM THROUGH ENTOMOPARASITES<br />
123<br />
CONCLUSIONS<br />
Basic <strong>and</strong> applied study of the EPN/bacteria symbiosis has increased steadily during<br />
the past half-century, coincident with an accelerating awareness of limitations that<br />
characterize many conventional pest management practices. An extensive literature<br />
on the effectiveness of EPNs as biopesticides is in striking contrast to the paucity of<br />
information about the ecology of these cryptic predators of subterranean arthropods.<br />
Their population abundance is usually inferred from the numbers of sentinel insects<br />
they kill but, unlike plant parasitic <strong>and</strong> free living nematodes, there are few reports<br />
of the actual numbers of these worms in different soil habitats. Consequently, little<br />
is known about their population biology – neither the factors that govern population<br />
size nor the numbers of worms needed to achieve economic pest suppression in<br />
different habitats. The great variety of species with very different life strategies<br />
provides tremendous opportunities to study how food webs <strong>and</strong> soil conditions<br />
affect the abundance of nematodes with different traits. Underst<strong>and</strong>ing the<br />
population biology of EPNs is necessary to discover <strong>and</strong> exploit new ways to<br />
increase their efficacy <strong>and</strong>, more importantly, their reliability for biological control<br />
in managed ecosystems. For example, trophic cascades that result from augmenting<br />
EPNs in citrus orchards have the potential to interfere with the effectiveness of this<br />
IPM tactic if the non-target effect (i.e., the temporary suppression of EPNs <strong>by</strong><br />
natural enemies) occurs at a peak time for D. abbreviatus egg hatch <strong>and</strong> larval<br />
recruitment into soil. Can better timing of EPN applications reduce this risk? Would<br />
the application of EPN species less susceptible to predation <strong>by</strong> NF modulate the<br />
trophic cascade <strong>and</strong> the potential for non-target effects? What physical<br />
characteristics of soils are amenable to change in ways that enhance either the<br />
numbers or the effectiveness of EPN? The ready availability of molecular tools to<br />
identify <strong>and</strong> measure EPN <strong>and</strong> their natural enemies in the soil should facilitate<br />
more rapid progress in our underst<strong>and</strong>ing of how these <strong>org</strong>anisms co-exist <strong>and</strong> how<br />
we might better manage soils to maximize their biological control potential.<br />
ACKNOWLEDGEMENTS<br />
The authors gratefully acknowledge postdoctoral fellowship support from the<br />
Ramón Areces Foundation (Spain) to R. Campos-Herrera <strong>and</strong> a US-Egypt project<br />
for IPM in citrus (contract 260) to L. W. Duncan.<br />
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Smith, M. E., & Jaffee, B. A. (2009). PCR primers with enhanced specificity for nematode-trapping fungi<br />
(Orbiliales). Microbial Ecology, 58, 117–128.<br />
Spiridonov, S. E., Reid, A. P., Podrunka, K., Subbotin, S. A., & Moens, M. (2004). Phylogenetic<br />
relationships within the genus Steinernema (Nematoda: Rhabditida) as inferred from analyses of<br />
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Stansly, P. A., Mizell, R. F., & McCoy, C. W. (1997). Monitoring Diaprepes abbreviatus with Tedder’s traps<br />
in Southwest Florida citrus. Proceedings of the Florida State Horticultural Society, 110, 22–26.<br />
Stirling, G. R., Griffin, D., Ophel-Keller, K., McKay, A., Hartley, D., Curran, J. et al. (2004). Combining<br />
an initial risk assessment process with DNA assays to improve prediction of soilborne diseases<br />
caused <strong>by</strong> root-knot nematode (Meloidogyne spp.) <strong>and</strong> Fusarium oxysporum f. sp. lycopersici in the<br />
Queensl<strong>and</strong> tomato industry. Australasian Plant Pathology, 33, 285–293.<br />
Stuart, R. J., Barbercheck, M. E., Grewal, P. S., Taylor, R. A. J., & Hoy, C. W. (2006). Population biology of<br />
entomopathogenic nematodes: Concepts, issues, <strong>and</strong> models. Biological Control, 38, 80–102.<br />
Stuart, R. J., El-Borai, F. E., & Duncan, L. W. (2008). From augmentation to conservation of<br />
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Subbotin, S. A., Madami, M., Krall, E., Sturhan, D., & Moens, M. (2005). Molecular diagnostics,<br />
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Timper, P., & Kaya, H. K. (1989). Role of the 2nd-stage cuticle of entomogenous nematodes in<br />
preventing infection <strong>by</strong> nemathophagus fungi. Journal of Invertebrate Pathology, 54, 314–321.<br />
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1262.
Section 2<br />
ADVANCED IPM TECHNOLOGIES
6<br />
INTEGRATION OF INSECT AND MITE<br />
MANAGEMENT WITH DISEASE AND WEED<br />
CONTROL IN PECAN PRODUCTION<br />
JAMES D. DUTCHER 1 , LENNY WELLS 2 , TIMOTHY B.<br />
BRENNEMAN 3 AND MICHAEL G. PATTERSON 4<br />
1 Entomology Department, University of Ge<strong>org</strong>ia, Tifton, GA, USA<br />
2 Horticulture Department, University of Ge<strong>org</strong>ia, Tifton, GA, USA<br />
3 Plant Pathology Department, University of Ge<strong>org</strong>ia, Tifton, GA, USA<br />
4 Department of Agronomy <strong>and</strong> Soils, Auburn University, Auburn, AL, USA<br />
Abstract. Pecan orchards in the southeastern US are managed to conserve resources, protect the fruit <strong>and</strong><br />
foliage from injury caused <strong>by</strong> phytophagous insects, mites, <strong>and</strong> pecan scab, <strong>and</strong> remove competition from weeds<br />
during the establishment of newly planted trees <strong>and</strong> in the preparation of the orchard floor as a harvesting<br />
surface. Costs associated with pest control are significant each year <strong>and</strong> the growers use integrated pest<br />
management methods to increase the effectiveness of pesticide treatments <strong>and</strong> reduce control costs. A<br />
coordinated research <strong>and</strong> extension effort over the past 25 years in entomology, plant pathology, weed science<br />
<strong>and</strong> horticulture has reduced the amount of pesticide use <strong>by</strong> 35%. Four advances have been responsible for the<br />
reduction. First, pecan scab sprays are reduced <strong>by</strong> linking the frequency of applications to the climatic conditions<br />
<strong>and</strong> the cultivar susceptibiltiy. Second, pest-specific insecticides that are toxic to the pests <strong>and</strong> not toxic to<br />
beneficial insects <strong>and</strong> mites are used to control lepidopterous pests <strong>and</strong> conserve aphidophagous insects <strong>and</strong> mite<br />
predators. Third, cover crops have been developed to supplement the soil with nitrogen <strong>and</strong> <strong>org</strong>anic matter <strong>and</strong><br />
conserve beneficial insects. Fourth, weed studies have led to the elimination of weeds in the first 8 years after<br />
planting around young trees, chemical mowing methods in established orchards <strong>and</strong> selective grass control to<br />
increase the growth of clover cover crops. The development <strong>and</strong> implementation of these <strong>and</strong> other significant<br />
advances in pecan management are reviewed in this chapter.<br />
1. PESTS IMPEDE THE VERSATILITY OF THE PECAN TREE<br />
Pecan [Carya illinoinensis (Wangenh.) K. Koch, Fagales: Jugl<strong>and</strong>aceae] is a large<br />
tree that is native to the United States <strong>and</strong> Mexico <strong>and</strong> is propagated as a shade tree,<br />
for timber <strong>and</strong> for the production of nuts. Although this chapter describes the recent<br />
integration of pest control methods in pecans grown for nut production pest<br />
problems arise in shade <strong>and</strong> timber trees as well. As a shade tree in the southern US,<br />
pecan has multiple problems <strong>and</strong> is not recommended for planting (Finch, 2001).<br />
However, existing trees are rarely removed <strong>and</strong> replaced <strong>by</strong> homeowners or city<br />
133<br />
A. <strong>Ciancio</strong>, K.G. Mukerji (eds.), Integrated Management of Arthropod Pests<br />
<strong>and</strong> Insect Borne Diseases, Integrated Management of Plant Pests <strong>and</strong> Diseases 5,<br />
DOI 10.1007/978-90-481-8606-8_6, © Springer Science+Business Media B.V. 2010
134<br />
J.D. DUTCHER ET AL.<br />
managers. The canopy of a full grown tree, with dimensions of 30.5 m in height <strong>and</strong><br />
16.5 m in diameter <strong>and</strong> covering up to 1/24 ha of l<strong>and</strong>, is often too large for home<br />
sites. The main pests of pecan trees planted along the roadside <strong>and</strong> in the urban<br />
l<strong>and</strong>scape, are the gregarious caterpillars – walnut caterpillar [Datana integerrima<br />
(Grote & Robinson), Lepidoptera: Notodontidae] <strong>and</strong> fall webworm [Hyphantria<br />
cunea Drury, Lepidoptera: Arctiidae]. These cause defoliation in the late summer<br />
<strong>and</strong> the fall webworm leaves unsightly webs in the canopy. Biological control with<br />
water-miscible formulations Bacillus thuringiensis applied as a foliar spray is<br />
effective against these two pests. Feeding <strong>by</strong> the pecan aphids [Monellia caryella<br />
(Fitch), Monelliopsis pecanis (Bissell), Melanocallis caryaefoliae (Davis),<br />
Hemiptera: Aphididae] also detract from the aesthetic value of pecan as a shade tree.<br />
Aphids egest copious amounts of honeydew (Wood, Tedders & Dutcher, 1987).<br />
Honeydew deposited on the leaf surface promotes the growth of sooty mold giving<br />
the leaves a black appearance. Honeydew deposited on the area beneath the tree<br />
canopy often has to be washed off cars <strong>and</strong> trucks parked beneath the trees.<br />
Multicolored Asian ladybeetle [Harmonia axyridis (Pallas), Coleoptera:<br />
Coccinellidae] was imported for biological control to the US <strong>and</strong> is an effective<br />
control for aphids in pecan trees in areas where the beetle is established. In pecan<br />
trees grown for shade, the nut crop is highly depredated <strong>by</strong> squirrels, birds <strong>and</strong> insect<br />
pests (Worley, 2002).<br />
Pecan lumber is sold as hickory <strong>and</strong> hickory is used to make tool h<strong>and</strong>les,<br />
furniture, cabinetry, ladder rungs, dowels, sporting goods (including baseball bats, skis<br />
<strong>and</strong> archery equipment), flooring, veneer, plywood, fuelwood, <strong>and</strong> charcoal. Pecan<br />
burls <strong>and</strong> spalted pecan are sold as a specialty wood. The characteristics of hickory<br />
<strong>and</strong> pecan produce a strong, shock-resistant wood that has a white tinge with brown<br />
sapwood <strong>and</strong> red-brown heartwood. Pecan wood is difficult to season <strong>and</strong> warps<br />
during drying. Wood working properties are above average for hickory <strong>and</strong> slightly<br />
less for pecan. Problems arise in splitting while nailing. Machining <strong>and</strong> glueing the<br />
wood are also difficult <strong>and</strong> the wood is susceptible to bird peck. Pest populations are<br />
generally very low in native st<strong>and</strong>s of pecan harvested for timber (Reid & Hunt, 2000).<br />
Yellow-bellied sapsucker, [Sphyrapicus varius (L.) Piciformes: Picidae] is a<br />
migratory bird that causes bird peck in hardwoods including pecan. The birds eat<br />
insects that are attracted to sap flowing from the holes made in the trunk <strong>by</strong> the bird<br />
pecks. Open bird peck holes do not decrease the value of the wood for lumber but<br />
they do devalue the wood used for making tool h<strong>and</strong>les. When the bird peck holes<br />
pierce the cambium layer of the trunk then the tree produces a callus tissue to repair<br />
the hole (aka an occlusion) <strong>and</strong> the wood looses value. Each yellow-bellied<br />
sapsucker returns to the same nesting site each year <strong>and</strong> repeated annual bird peck<br />
damage can extend into the wood <strong>and</strong> reduce its value. Foresters control the yellowbellied<br />
sapsucker <strong>by</strong> applying bird Tanglefoot® on the trunk of most of the trees in<br />
the orchard leaving a few favored trees untreated to withst<strong>and</strong> all the injury. The<br />
birds nest in decaying trunks of aspen <strong>and</strong> removal of these nesting sites also<br />
reduces injury. Killing the birds is illegal (Ostry & Nicholls, 1978). Pecan are also<br />
be used as an alley crop in the southern US. The trees are planted around fields of<br />
row crops <strong>and</strong> the tree roots reduce nitrate leaching from the crop field to the<br />
groundwater (Allen et al., 2004).
IPM IN PECAN PRODUCTION<br />
135<br />
Pecan nut production in orchards is a viable agribusiness especially in the<br />
southern US. Pecan trees will produce a crop of nuts with little or no management.<br />
In fact, a large portion of the USA crop is produced on native st<strong>and</strong>s with very low<br />
inputs. These st<strong>and</strong>s have much lower average production per hectare than seedling<br />
or improved pecan orchards <strong>and</strong> inputs have to be held to a low cost. Pecans initially<br />
were harvested <strong>by</strong> h<strong>and</strong>. Harvesters would climb each tree <strong>and</strong> shake individual<br />
limbs or knock nuts off the limbs with bamboo poles, while coworkers would pick<br />
them up off the ground. Mechanical trunk <strong>and</strong> limb shakers are currently used to<br />
dislodge the nuts out of the tree <strong>and</strong> onto the orchard floor. H<strong>and</strong> picking off the<br />
ground has been replaced <strong>by</strong> a mechanical process where the fallen limbs are raked<br />
over to the edge of the orchard, the nuts <strong>and</strong> leaves are swept into rows, the leaves<br />
are blown off the row <strong>and</strong> the nuts are picked up from the row <strong>by</strong> a mechanical<br />
harvester. Nuts are sorted <strong>and</strong> cleaned in the orchard <strong>and</strong> then transported to the<br />
shelling plant where they are sanitized, dried <strong>and</strong> then typically cracked, shelled <strong>and</strong><br />
frozen. Harvesting is most efficient when the orchard floor is dry, level, <strong>and</strong> cleared<br />
of weeds <strong>and</strong> debris. Efficient harvesting is needed to prevent depredation of the<br />
nuts <strong>by</strong> birds <strong>and</strong> mammals <strong>and</strong> environmental degradation of the nuts.<br />
Native st<strong>and</strong>s of pecans provided nuts as a source of food for indigenous<br />
people of America <strong>and</strong> early settlers propagated seedling trees through the southern<br />
US. Many of the native groves were developed, <strong>by</strong> European settlers, as a newworld<br />
adaptation (Brison, 1974) of the European silvopastoral systems that provided<br />
many of the staples of the rural community – milk, meat, hides, wood, <strong>and</strong> nuts<br />
(Auda, 1999). Grafting techniques were developed in the mid-1800s <strong>and</strong> improved<br />
cultivars with desirable characteristics were selected from native <strong>and</strong> seedling trees<br />
or from controlled crosses from amateur or professional plant breeders. Improved<br />
cultivars have been propagated across the southeastern US, <strong>and</strong> in New Mexico,<br />
Arizona <strong>and</strong> California to the extent that the production of nuts from improved<br />
cultivars often exceeds the production of native <strong>and</strong> seedling orchards (Worley,<br />
2002).<br />
Nut production in the US is currently based on ~10 million managed trees<br />
planted on ~200,000 ha on 20,000 farms in 24 states producing roughly 146,000<br />
metric tons of in-shell nuts each year. Most orchards are small in area. Sixty-two<br />
percent of the farms have less than 6 ha, 32% have 6–40 ha, 5.4% of the farms have<br />
40–200 ha <strong>and</strong> 0.7% of the farms have more than 200 ha. Orchards with less than 40<br />
ha comprise 56% of the production area in the USA (Wood, 2003). Improved<br />
cultivars have contributed to increases in pecan production. Today’s new cultivars,<br />
however, are only 2–3 generations removed from wild trees (Sparks, 1992) <strong>and</strong><br />
pesticides – esp. fungicides – have had a more significant impact on increasing USA<br />
pecan production than cultivars. In fact, native groves produce approximately 30%<br />
of the US nut crop <strong>and</strong> seedling <strong>and</strong> improved cultivars planted in commercial<br />
orchards produce the remaining crop (Pollack, 2001). Pecan trees have a producing<br />
lifespan of at least 80 years <strong>and</strong> grow to over 30.5 m in height. Production is<br />
irregular from season to season. USA production per season ranges from 45.4<br />
to 163.2 million kg of nuts in the shell. The kernel typically comprises ~50%<br />
of the mass of the nut in the shell. Growers typically sell pecans in the shell for<br />
$1.50–5.00/kg to processors <strong>and</strong> many growers process, package, <strong>and</strong> market their
136<br />
J.D. DUTCHER ET AL.<br />
own crop as higher value products such as gift boxes, whole kernels, <strong>and</strong> various<br />
c<strong>and</strong>ies. Growers in Ge<strong>org</strong>ia <strong>and</strong> Texas produce 60% of the US crop.<br />
2. PEST CONTROL METHODS<br />
Uncontrolled disease, insect <strong>and</strong> mite, <strong>and</strong> weedy pest populations, under favorable<br />
environmental conditions have the potential of reducing the pecan nut production<br />
often to nil. Pests attacking the nuts can take the entire crop in the current season.<br />
Pests attacking the foliage can cause premature defoliation in the current year <strong>and</strong><br />
the trees will not produce flowers <strong>and</strong> fruit the following year As examples, the<br />
primary pest in the humid regions of the southeastern US is pecan scab <strong>and</strong> control<br />
is achieved with preventive treatment of the fruit <strong>and</strong> foliage with fungicide. Pecan<br />
weevil attacks the crop late in the season after the grower has invested considerable<br />
resources in the crop <strong>and</strong> the weevils are most effectively controlled with repeated<br />
sprays of insecticide during adult emergence. Black pecan aphid outbreaks defoliate<br />
trees quickly <strong>and</strong> treating after the outbreak does not prevent damage. Black pecan<br />
aphids are treated with insecticide when the population exceeds one aphid per leaf.<br />
Pecan leaf scorch mite is control with sprays of sulphur or miticide (Dutcher,<br />
Hudson & Ellis, 2003). Lack of weed control is directly related reductions in pecan<br />
production, esp. in young pecan trees (Smith, Cheary, & Carroll, 2005; Patterson &<br />
Goff, 1993; Foshee, Goodman, Patterson, Goff, & Dozier, 1997).<br />
Broad spectrum pesticides <strong>and</strong> airblast sprayer technology <strong>and</strong> orchard floor<br />
management significantly increase the ability of growers to quickly control these<br />
key pests <strong>and</strong> large portions of the nut crop were conserved <strong>by</strong> the use the pesticides.<br />
Production of nuts increased leading to a period of reliance on chemical control of<br />
insects, mites <strong>and</strong> diseases. Broad spectrum pesticides are crucial to commercial<br />
pecan production, offering highly effective control methods that prevent pecan scab<br />
<strong>and</strong> pecan weevil damage, control outbreaks of black pecan aphids, <strong>and</strong> prepare<br />
weed-free herbicided strips along the tree rows.<br />
Pest control in differs in each of the three cultural regimes for pecan nut<br />
production (Dutcher et al., 2003). In native st<strong>and</strong>s <strong>and</strong> groves where nuts are<br />
harvested from naturally occurring trees, the orchard floor is cleared at harvest time<br />
<strong>and</strong> the nuts are collected <strong>and</strong> managers use nitrogen fertilization, mechanical nut<br />
harvest rely primarily on natural controls to regulate pest populations with limited<br />
use of insecticides (Reid & Mulder, 2003). In seedling orchards where trees are<br />
produced from seed <strong>and</strong> not grafted, <strong>and</strong> in improved orchards where seedlings are<br />
grafted in a nursery to a known cultivar <strong>and</strong> then planted in an orchard, orchard<br />
managers potentially can use all available pest control methods <strong>and</strong> are limited <strong>by</strong><br />
the need to balance the costs of control with production potential each season. Each<br />
seedling tree produces a unique pecan nut <strong>and</strong> the harvested product lacks the<br />
homogeneity of the nut crop harvested from an improved orchard. However,<br />
seedling orchards have greater genetic diversity than improved orchards <strong>and</strong> pest<br />
outbreaks (especially for pecan scab, pecan weevil <strong>and</strong> black pecan aphid) develop<br />
to different levels of severity in each tree. Improved orchards are more susceptible to<br />
pest outbreaks over the entire orchard.
IPM IN PECAN PRODUCTION<br />
137<br />
Weed control is important <strong>and</strong> functions to: remove plants that compete with<br />
the trees for nutrients <strong>and</strong> plants that provide food for kernel-feeding hemipterans;<br />
<strong>and</strong>, to the preparation of the orchard floor for mechanical harvesting (Smith &<br />
Carroll, 2004). Weed control initially consisted of disking <strong>and</strong> rolling the soil so that<br />
the nuts could be collected from bare soil surface. This method made harvesting<br />
easier but the harrow would often open a wound at the base of the trunk of each tree<br />
<strong>and</strong> crown gall [Agrobacterium tumefaciens Smith & Townsend, Proteobacteria:<br />
Rhizobiales: Rhizobiaceae] would infest the wounded trees <strong>and</strong> destroy a fair<br />
portion of the root system. Growers shifted to a mowed surface between tree rows<br />
with an herbicided strip along the tree row to prevent damage to the tree trunks.<br />
Through the years the types of herbicides changed but the basic design remained the<br />
same. Trees on l<strong>and</strong> that is flooded part of the year along river systems or with flood<br />
irrigation have either a bare soil surface maintained with herbicides or the annual<br />
weeds are periodically mowed. In the last 30 years, growers have started an<br />
integrated approach to weed control <strong>by</strong> seeding the orchard with various cool season<br />
legumes. These are grown as intercrops in the mowed strip or as cover crops over<br />
the entire orchard floor. The plants supply nitrogen <strong>and</strong> increase soil <strong>org</strong>anic matter<br />
<strong>and</strong> also enhance beneficial insects. In the last 5 years, growers have enhanced the<br />
growth of the legumes <strong>by</strong> removing grasses during the winter <strong>and</strong> spring with,<br />
sethoxydim, a selective herbicide.<br />
Agricultural chemical usage in US pecan orchards varies considerably between<br />
states <strong>and</strong> has increased significantly since the domestication of pecan began in the<br />
early 1900s. Nitrogen fertilizer, pesticides <strong>and</strong> new cultivars have increased US<br />
production per hectare. Pesticide usage is significant, for example, commercial<br />
pecan producers currently use approximately 1/3 million kg of insecticide (active<br />
ingredient) each season on 320,000 acres in Ge<strong>org</strong>ia <strong>and</strong> Texas (Smith, Harris, Lee,<br />
McEachern, & Ree, 2002; Guillebeau, 2001). The most recent survey results<br />
(USDA/NASS, 2000) indicate that approximately 69% of the US pecan acreage is<br />
treated each year with supplemental nitrogen fertilizer, 67% is treated with<br />
insecticides, 47% is treated with fungicides, <strong>and</strong> 44% is treated with herbicides.<br />
2.1. Insect <strong>and</strong> Mite Pest Management in Pecan Orchards<br />
The insect complex associated with pecan in native <strong>and</strong> improved systems includes<br />
180 species of phytophagous insects <strong>and</strong> mites (Payne & Johnson, 1979; Harris,<br />
1983) <strong>and</strong> each is associated <strong>by</strong> a diverse array of natural enemies (Tedders, 1985).<br />
Insect management strategies range from total reliance on natural enemies to<br />
intensive integration of chemical <strong>and</strong> biological controls (Table 1) (Dutcher et al.,<br />
2003). The fruit <strong>and</strong> foliage in pecan orchards are susceptible to insect injury that<br />
can result in economic losses for 7 months. Preventive cover sprays of insecticides<br />
or miticides are not practical <strong>and</strong> the control of pecan insect <strong>and</strong> mite pests has<br />
developed into a management scheme. Insects <strong>and</strong> mites <strong>and</strong> tree phenology are<br />
monitored determine the abundance of the pests <strong>and</strong> the susceptibility of the tree to<br />
injury. Direct control measures are applied when pest abundance exceeds an action<br />
threshold <strong>and</strong> the tree is susceptible to injury. This prevents high costs, resistance,
138<br />
J.D. DUTCHER ET AL.<br />
replacement <strong>and</strong> resurgence problems associated with repeated treatment with<br />
insecticides <strong>and</strong> miticides (Dutcher, Fonsah, & Hudson, 2006).<br />
Table 1. Control methods for the eight major pecan arthropod pests in North American.<br />
Pest Control method for pest a Relative efficacy b<br />
Pecan weevil<br />
Curculio caryae (Horn)<br />
Pecan nut casebearer<br />
Acrobasis nuxvorella (Neunzig)<br />
Hickory shuckworm<br />
Cydia caryana Fitch<br />
Black pecan aphid<br />
Melanocallis caryaefoliae Davis<br />
Yellow pecan aphid<br />
Monelliopsis pecanis Bissell<br />
Blackmargined aphid<br />
Monellia caryella Fitch<br />
Pecan leaf scorch mite<br />
Eotetranychus hicoriae<br />
(McGregor)<br />
Kernel-feeding Hemipterans –<br />
Pentatomidae <strong>and</strong> Coriedae<br />
Broad spectrum insecticides<br />
Quarantine<br />
Risk rating <strong>and</strong> spot treatment<br />
Trunk treatment<br />
Entomopathogens, nematodes<br />
Red imported fire ant as predator<br />
Broad spectrum insecticides<br />
Biorational insecticides<br />
Mating disruption<br />
Broad spectrum insecticides<br />
Biorational insecticides<br />
Sanitation<br />
Organophosphate insecticides<br />
Neonicitinoid insecticides<br />
Insecticidal soap<br />
Harmonia axyridis (Pallas)<br />
Interplanting crape myrtles<br />
Systemic insecticides<br />
Neonicitinoid insecticides<br />
Insecticidal soap<br />
Harmonia axyridis (Pallas)<br />
Introduced parasites<br />
Systemic insecticides<br />
Neonicitinoid insecticides<br />
Insecticidal soap<br />
Harmonia axyridis (Pallas)<br />
Introduced parasites<br />
Miticides<br />
Sulphur<br />
Predatory mite release<br />
Dormant oil sprays<br />
Broad spectrum insecticides<br />
Trap crops<br />
Removing alternate host plants<br />
High<br />
High<br />
Moderate<br />
Moderate<br />
Low<br />
Low<br />
High<br />
High<br />
Low<br />
High<br />
High<br />
Moderate<br />
High<br />
Moderate<br />
High<br />
Moderate<br />
Low<br />
High<br />
High<br />
High<br />
Low<br />
Low<br />
High<br />
High<br />
High<br />
Low<br />
Low<br />
High<br />
High<br />
Moderate<br />
Low<br />
Moderate<br />
Low<br />
Low<br />
a<br />
b<br />
Control methods listed in the table have shown benefits greater than the costs.<br />
Efficacy ratings: total = 100%; high = 91–100%; moderate = 80–90%; low < 80%.<br />
Insecticides offer the single most effective control method for nut-feeding<br />
insects. Carbaryl, phosmet, esfenvalerate <strong>and</strong> cypermethrin are used during the late<br />
season for control of pecan weevil, hickory shuckworm <strong>and</strong> kernel-feeding
IPM IN PECAN PRODUCTION<br />
139<br />
hemipterans. Pyrethroid insecticides are also used but have a shorter residual activity<br />
<strong>and</strong> lower toxicity against the pecan weevil. Broad spectrum insecticides are not<br />
ideal <strong>and</strong> sprays often destroy beneficial insects leading to resurgence of secondary<br />
foliage-feeding pests. Pecan growers with resurgence problems have to apply<br />
additional costly <strong>and</strong> specific aphidicides, systemic insecticides <strong>and</strong>/or miticides to<br />
keep the foliage on the trees.<br />
Systemic insecticides or foliar sprays of insecticides are the most effective<br />
controls for outbreaks of foliage feeding insects. Phosmet <strong>and</strong> chlorpyrifos are used<br />
effectively for control of late season outbreaks of the black pecan aphid. These two<br />
<strong>org</strong>anophosphate insecticides may become obsolete through reassessment.<br />
Imidacloprid sprays <strong>and</strong> biological control with multicolored Asian ladybeetle are<br />
effective against the pecan aphids. Efficacy varies between the three different<br />
species <strong>and</strong> selective control of two aphid species <strong>and</strong> not the third species opens the<br />
feeding niche the third leading to outbreaks. The control of all three species of pecan<br />
aphids can leave the foliage open to attack <strong>by</strong> phytophagous mites <strong>and</strong> typically<br />
leads to an outbreak of pecan leaf scorch mite (Dutcher et al., 2006). Alternative<br />
controls for control of nut-feeding pests that do not destroy beneficial insects<br />
associated with foliage-feeding pests are possible with the use of selective<br />
insecticides.<br />
Growers also adopt insect pest management to reduce the cost of production for<br />
pecans. Pecan growers typically minimize the number of spray applications <strong>and</strong> rely<br />
on natural control <strong>by</strong> predators, parasites <strong>and</strong> pathogens for many insect pests. One of<br />
the most effective biologically-based control techniques for pecan growers is selective<br />
insecticides coupled with effective monitoring techniques. to control pecan nut<br />
casebearer (Knutson & Ree, 2000) <strong>and</strong> hickory shuckworm. Replacement of broad<br />
spectrum insecticides with biorational insecticides has reduced the incidence of<br />
secondary pest resurgence after treatments for these pests. Initially, insect growth<br />
regulators were evaluated for insect control against pecan weevil <strong>and</strong> lepidopterans<br />
(Payne & Dutcher, 1985; Tedders, 1977). Efficacy was much lower than the broadspectrum<br />
insecticides <strong>and</strong> registration was not pursued. Broad-spectrum insecticides<br />
became the main control measures for preventing pest damage. Recently, newer <strong>and</strong><br />
more effective insect growth regulator insecticides, such as, diflubenzuron <strong>and</strong><br />
tebufenozide, have gained acceptance among growers for control of lepidopteran<br />
pests. Broad spectrum insecticides are currently the only effective controls for pecan<br />
weevil, kernel-feeding hemipterans <strong>and</strong> black pecan aphid.<br />
Pecan insects have sufficient reproductive capacities to overcome the mortality<br />
caused <strong>by</strong> control methods <strong>and</strong> growers are continually battling recurring pest<br />
problems each season. The bionomics information for the reproductive capacity <strong>and</strong><br />
generation time of pecan weevil (Ree, Knutson, & Harris, 2005), pecan nut<br />
casebearer (Mulder & Grantham, 2002), yellow pecan aphid, blackmargined aphid,<br />
black pecan aphid (Tedders, 1978; Kaakeh & Dutcher, 1992), <strong>and</strong> pecan leaf scorch<br />
mite (Hall, 2001) (Table 2) indicates that only 0.1–70% of the populations need to<br />
survive from one season to the next to sustain the pest populations.<br />
Pecan weevil survival of 2.6% per generation is needed to sustain the current<br />
population level. Since there is a generation every 2–3 years, an annual mortality of<br />
30.1% per season (for weevils with a 3-year generation time) or 83.4% per season
140<br />
J.D. DUTCHER ET AL.<br />
(for weevils with a 2-year generation time) would cause a decrease in weevil from<br />
one generation to the next. Multiple generations occur for pecan nut casebearer,<br />
aphids <strong>and</strong> pecan leaf scorch mite <strong>and</strong> yearly survivals of 0.1–0.2% will ensure a<br />
increase in theses pest populations from season to season. Efficacies required to<br />
prevent pecan nut casebearer populations from increasing from season to season<br />
exceed 99% <strong>and</strong> two or more control methods often have to be combined to prevent<br />
pest outbreaks in an integrated pest management program (cf. Tables 1 <strong>and</strong> 2). The<br />
better chemical control methods typically have efficacies near 95–99%. The impacts<br />
of natural controls – e.g. rainfall events (Kaakeh & Dutcher, 1993a) <strong>and</strong> temperature<br />
extremes (Kaakeh & Dutcher, 1993b) on pecan aphids – are important but pests also<br />
may increase in the orchard <strong>by</strong> immigration. Consequently, growers continue to<br />
have pest problems from season to season. Pecan weevil problems may be solvable<br />
with the integration of several techniques over an extended period.<br />
Table 2. The mortality needed each season to cause a reduction in the season to season<br />
abundance estimated from literature values for the reproductive capacity (RC) <strong>and</strong><br />
generations per year (G), for certain pecan insect <strong>and</strong> mite pests with the equation:<br />
Mortality (%) = 100 ⋅ (1 – (1 / (SR ⋅ RC) G )), where the sex ratio (SR) is assumed to be<br />
1.0 for aphids <strong>and</strong> 0.5 for weevils, casebearers <strong>and</strong> mites.<br />
Pest a Reproductive capacity Generations<br />
per year<br />
Mortality<br />
per season (%)<br />
Pecan weevil 75 eggs/female 0.3– 0.5 30–83<br />
Pecan nut casebearer 50–150 eggs/female 2 99.8–99.9<br />
Black pecan aphid 35 nymphs/female 26 99.9<br />
Yellow pecan aphid 38 nymphs/female 32 99.9<br />
Black margined aphid 125 nymphs/female 16 99.9<br />
Pecan leaf scorch mite 9–36 eggs/female 7-8 99.9<br />
a Two pest listed in Table 1 are not listed here. The reproductive capacity of the hickory shuckworm has<br />
not been measured <strong>and</strong> the moths have 2–5 generations per year. Kernel-feeding hemipterans do not<br />
reproduce in the pecan trees <strong>and</strong> increases in abundance <strong>by</strong> immigrating from alternative host plants.<br />
2.2. Pecan Disease Management<br />
There are multiple diseases of pecan that can impact production <strong>by</strong> reducing yield or<br />
quality of nuts in the present year, or reducing the ability of the trees to produce in<br />
subsequent seasons. This is particularly true in the southeastern US where fungal<br />
diseases thrive in the warm, humid climate present during the growing season.<br />
Production areas of the western US have much drier climates <strong>and</strong> few problems with<br />
fungal diseases. Therefore most of the following comments will pertain to disease<br />
control practices in the wetter production areas from east-central Texas through<br />
South Carolina. In this region the most damaging disease <strong>by</strong> far is pecan scab caused
IPM IN PECAN PRODUCTION<br />
141<br />
<strong>by</strong> Fusicladosporium effusum (G. Winter) Partridge <strong>and</strong> M<strong>org</strong>an-Jones. Most years<br />
disease losses are not that high, but growers often spend more money for fungicides<br />
than any other production input. In Ge<strong>org</strong>ia alone the cost of scab control is<br />
estimated to be about $15 million annually, <strong>and</strong> in a wet year like 2003 the<br />
combined cost of lost yield <strong>and</strong> fungicide sprays was approximately $45 million<br />
(Williams-Woodward, 2003). There are other diseases that can cause local damage<br />
on some cultivars, but they are generally controlled <strong>by</strong> fungicides applied for scab.<br />
These secondary diseases include Downy Spot (Mycosphaerella caryigena),<br />
Phytopthora Shuck <strong>and</strong> Kernel Rot (Phytophthora cactorum), Powdery mildew<br />
(Microsphaera penicillata), Zonate leaf spot (Cristulariella pyrimidalis),<br />
Anthracnose (Glomerella cingulata), Bacterial leaf scorch (Xylella fastidiosa),<br />
Crown gall (Agrobacterium tumefaciens), <strong>and</strong> a number other minor diseases that<br />
rarely cause significant crop loss.<br />
Because losses to disease can be severe under favorable conditions, growers<br />
have a high awareness of the need for control programs. This may include practices<br />
such as pruning lower tree branches or clearing fence rows around orchards,<br />
planting in wide row spacing’s, closely mowing the orchard floor, <strong>and</strong> designing<br />
orchards so that prevailing winds flow through it (Latham & Goff, 1991). All these<br />
practices are designed to increase air flow, thus reducing leaf wetness periods <strong>and</strong><br />
therefore levels of infection. General orchard sanitation practices are also utilized,<br />
<strong>and</strong> may include shaking previously harvested trees to dislodge shucks that harbor<br />
overwintering pathogen inoculum.<br />
In spite of these practices, growers in areas with frequent rainfall rely heavily<br />
on multiple fungicide applications applied with large air-blast sprayers or<br />
occasionally airplanes. Fungicides used include triphenyltin hydroxide (TPTH),<br />
various sterol demethylation inhibitors (DMI’s), dodine, strobilurins, <strong>and</strong><br />
thiophanate methyl. There have been issues recently with fungicide resistance, <strong>and</strong><br />
ongoing concerns that it will become an increasing problem (Stevenson, Bertr<strong>and</strong>, &<br />
Brenneman, 2004). These concerns are based on the known risks associated with the<br />
fungicides used, the inherent ability of the pathogen to develop resistance, the heavy<br />
use of fungicides, <strong>and</strong> the fact that pecan is a perennial crop <strong>and</strong> therefore not<br />
subject to crop rotation which can greatly reduce the buildup of resistant isolates.<br />
However, growers generally still get good disease control if they apply sprays<br />
correctly <strong>and</strong> on a timely basis. Most growers in the southeastern states use a 2–3<br />
weeks spray interval for a total of 7–10 sprays per year, whereas those in more arid<br />
areas of the west may make few if any fungicide applications.<br />
Early sprays (i.e. prepollination) are applied to protect the young leaves which<br />
are very susceptible to scab infections. Overwintered lesions on stems are a major<br />
source of this initial inoculum. Large numbers of conidia are produced from stem<br />
lesions in late March <strong>and</strong> early April, although small numbers are found as late as<br />
August (Stevenson, 1995). Therefore one function of the early sprays is to prevent<br />
leaf infections that will in turn sporulate <strong>and</strong> provide secondary inoculum for nut<br />
infections that are even more damaging. Scab susceptibility of leaves decreases<br />
rapidly with age (Gottwald, 1985), although later season growth flushes can become<br />
infected. Late-season fungicide sprays are of questionable benefit when applied after<br />
shell hardening according to work <strong>by</strong> Gottwald <strong>and</strong> Bertr<strong>and</strong> (1989). They
142<br />
J.D. DUTCHER ET AL.<br />
demonstrated that scab initiated at this time of the season was largely cosmetic since<br />
it occurred after the nuts had fully exp<strong>and</strong>ed. However, many growers still apply<br />
fungicides at this time.<br />
In an effort to reduce the cost of production in areas prone to scab<br />
development, several programs have been developed to enable growers to spray only<br />
when the environmental conditions are conducive for disease development. The<br />
program currently recommended in Ge<strong>org</strong>ia is AU-Pecan which is based on the<br />
number of rainfall events as well as the predicted chance of rain for the next 5 days.<br />
This model has been shown to reduce the total number of sprays in most seasons<br />
while maintaining the same level of control, <strong>and</strong> is available on a site-specific basis<br />
for individual orchards using Doppler radar precipitation estimates. A different<br />
model based on scab hours, i.e. periods with temperatures > 21.1°C <strong>and</strong> relative<br />
humidity >90%, is being used in Oklahoma (Von Broembsen, Driever, Smith,<br />
Duthie, & Carlson, 1999). One limitation to implementation of any advisory is the long<br />
time needed for many growers to spray their orchards. This time frame is commonly 1–2<br />
weeks, which necessitates spraying on more of a calendar-based schedule since response<br />
to an advisory is too slow. The AU-Pecan model compensates for this to some degree <strong>by</strong><br />
utilizing the 5-day chance of rain to recommend applications prior to favorable infection<br />
periods, rather than waiting until after they occur.<br />
Another consideration in scheduling fungicide sprays based on scab biology<br />
alone is the potential development of other diseases. For example, Stuart has been a<br />
more scab-resistant cultivar in some areas <strong>and</strong> often receives fewer sprays than more<br />
scab-susceptible cultivars. However, it is very susceptible to downy spot. Downy spot<br />
infections occur very early in the season, <strong>and</strong> prepollination fungicide sprays are<br />
essential for control. The spectrum of activity for a given fungicide must also be<br />
considered when designing a spray program. A product must have activity on scab, but<br />
some excellent scab fungicides do not control other diseases as well. One common<br />
example of this is the lack of activity of TPTH <strong>and</strong> dodine on zonate leaf spot. Both of<br />
these fungicides provide excellent control of nut scab, but are weak on zonate leaf spot<br />
which also occurs during nut fill. In orchards where zonate can be a problem, other<br />
classes of fungicides (particularly DMI’s) should be incorporated into post-pollination<br />
spray programs to insure control of this potentially damaging disease.<br />
One problem that is exacerbated <strong>by</strong> fungicide sprays is pecan aphids. As<br />
discussed earlier, several species of aphid can be very detrimental to pecan, but there<br />
is a beneficial fungus in the Neozygitaceae that can cause high aphid mortality<br />
(Ekbom & Pickering, 1990). Unfortunately this fungus is very sensitive to TPTH,<br />
<strong>and</strong> fungal-induced aphid mortality was reduced <strong>by</strong> 50% in trees sprayed with this<br />
commonly used fungicide (Pickering, Dutcher, & Ekbom, 1990). Therefore,<br />
reductions in fungicide use not only save money, they also make it less likely that a<br />
grower will have to spray insecticides later in the year for aphid control (Pickering,<br />
Hargrove, Dutcher, & Ellis, 1990).<br />
Virulence of the pecan scab fungus has been shown to be very cultivar specific<br />
(Converse, 1960). Early researcher (Demaree & Cole, 1929) demonstrated that<br />
repeated inoculations on the same cultivar increased pathogenicity on that cultivar,<br />
<strong>and</strong> the history of scab-resistant cultivar introductions has consistently been that<br />
they become more susceptible to damaging scab epidemics each year (Gottwald,
IPM IN PECAN PRODUCTION<br />
143<br />
1989). The basis for this specificity is not fully known, but it occurs sometime later<br />
than 4 days after inoculation during the stage of subcuticular growth (Bracewell &<br />
Stevenson, 1999). Intercropping a mixture of cultivars has been shown to<br />
successfully reduce epidemics of foliar pathogens in other crops (Mundt, 2002), <strong>and</strong><br />
computer simulations based on apple scab show disease reductions of 65–79% after<br />
six generations when planting three cultivars versus a single cultivar (Gessler &<br />
Blaise, 1994). While utilizing that model to guide cultivar placement in new<br />
orchards has been discussed among pecan growers <strong>and</strong> researchers, the benefits of<br />
planting cultivars in blocks for other management purposes usually outweigh the<br />
potential benefits related to scab control.<br />
The race structure of pecan scab populations <strong>and</strong> their ability to adapt to new<br />
cultivars has raised questions regarding the objectives of pecan breeding programs<br />
which involve selecting for scab resistance. Breeders have selected for scab resistance<br />
for years, <strong>and</strong> there have also been attempts to introduce new resistance factors from<br />
other members of the hickory family via interspecific crosses (Graves & Diehl, 1991).<br />
It has generally been recognized that there is a “grace period” after the introduction of<br />
a new cultivar before scab becomes adapted to it, <strong>and</strong> the length of this grace period<br />
varies considerably among cultivars. One objective of the Ge<strong>org</strong>ia breeding program is<br />
to introduce new cultivars with high quality nuts with different resistance genes that<br />
can be transitioned into orchards to maintain diversity (Conner, 2003). The current<br />
Ge<strong>org</strong>ia program is also utilizing DNA markers for resistance genes <strong>and</strong> examining<br />
the physiological basis for scab resistance. Hopefully these efforts will lead to more<br />
durable field resistance in new pecan cultivars.<br />
2.3. Weed Management in Pecan Orchards<br />
Weeds are present throughout the world <strong>and</strong> many interfere with the optimum<br />
production of food <strong>and</strong> fiber. Holm, Doll, Holm, <strong>and</strong> Pancho (1997) state that<br />
approximately 200 plant species world wide are found to cause widespread<br />
problems in our crops. Many of these weeds occur in fruit <strong>and</strong> nut crops. Pecans are<br />
grown in the southern US <strong>and</strong> Mexico, an area that accounts for over 98% of the<br />
world’s pecan production (Pena, 2006). Vines, including annual vines such as the<br />
morningglories (Ipomoea species) <strong>and</strong> perennial vines such as trumpet creeper<br />
(Campsis radicans), <strong>and</strong> both annual <strong>and</strong> perennial grasses such as crabgrass<br />
(Digitaria spp.), goosegrass (Eleusine indica), bahiagrass (Paspalum notatum) <strong>and</strong><br />
bermudagrass (Cynodon dactylon), are some of the most common <strong>and</strong> troublesome<br />
weeds in pecans (Southern Weed Science Society, 2006). Other species commonly<br />
found in pecan orchards include nutsedge (Cyperus species), horsenettle (Solanum<br />
species), arrowleaf sida (Sida rhombifolia), spurges (Euphorbia species), horseweed<br />
(Conyza canadensis), <strong>and</strong> pigweed (Amaranthus species) Colour pictures <strong>and</strong><br />
descriptions are found in the Weed Identification Guide published <strong>by</strong> the Southern<br />
Weed Science Society (2007).<br />
Numerous weed-competition studies have shown the adverse effects of weeds<br />
on agronomic, vegetable, <strong>and</strong> fruit crops (Zimdahl, 2004). These studies generally<br />
document the effects of individual weed species on the growth <strong>and</strong>/or yield of a
144<br />
J.D. DUTCHER ET AL.<br />
crop. Density studies have determined the effect of increasing weed density in<br />
season-long competition with the crop. Period of competition studies have<br />
determined the length of time the crop can tolerate competition from a specific weed<br />
at a specific density without incurring yield loss; or conversely, how long the crop<br />
must be maintained free of this weed before it can produce an optimum crop.<br />
Different types of information can be obtained with these studies. The critical period<br />
of weed control (CPWC) has been defined <strong>by</strong> Knezevic, Evans, Blankenship, Van<br />
Acker, <strong>and</strong> Lindquist (2002), as the time interval between two measured crop-weed<br />
competition components: (i) the maximum amount of time early-season weed<br />
competition can be tolerated <strong>by</strong> the crop before a yield loss occurs, <strong>and</strong> (ii) the<br />
weed-free period required from planting to obtain optimum yield (independent of<br />
other confounding factors, i.e. late season drought, insects, diseases, etc.). This<br />
period has been shown to vary from zero up to several weeks in work done with<br />
annual crops <strong>and</strong> weeds (Knezevic et al., 2002). In layman terms this answers the<br />
questions; how long must I maintain weed control in the crop to obtain optimum<br />
growth <strong>and</strong> yield, or how late can I wait to initiate <strong>and</strong> maintain weed control<br />
without incurring yield loss? Because most of the weed-competition studies were<br />
conducted using annual crops grown in narrow spacings (< 1 m) competing with<br />
annual weeds, weed control measures were generally applied on a “broadcast” basis.<br />
This is generally not the case with weed management in pecan orchards.<br />
Current weed management in pecan orchards involves weed control within a<br />
narrow strip centered on the pecan tree row. Also, many of the most troublesome<br />
weeds in pecan orchards are perennials. The CPWC has never been determined for<br />
pecan <strong>and</strong> would probably take several years research to determine. Smith (1999)<br />
determined that substantial reduction in growth of pecan trees occurred <strong>by</strong> weed<br />
competition from cutleaf eveningprimrose (Oenothera laciniata), a cool-season<br />
species, implying that the presence of weeds results in reduced growth of pecans<br />
even in cool months.<br />
Although several methods of orchard floor management have been used in the<br />
past, including mowing <strong>and</strong> cultivation (Ark, 1954), the use of registered herbicides<br />
is currently the most common method used <strong>by</strong> far (Alabama Cooperative Extension<br />
System, 2007; Ge<strong>org</strong>ia Cooperative Extension Service, 2007; Smith & Carroll,<br />
2004). Herbicidal active ingredients used to maintain weed control in pecan orchards<br />
include oryzalin, pendimethalin, diuron, simazine, norflurazon, fluazifop,<br />
sethoxydim, clethodim, flumioxazin, halosulfuron, paraquat, glufosinate,<br />
glyphosate, <strong>and</strong> carfentrazone. These herbicides can be used at different times <strong>and</strong><br />
for specific weeds in orchard floor management. Some are restricted to non-bearing<br />
trees only, <strong>and</strong> some to trees established at least 2–3 years in the orchard. Most<br />
orchard floor management programs use a combination of these products to<br />
maintain season-long control in a weed-free strip centered on the tree row.<br />
Combinations of registered herbicides used in both preemergence <strong>and</strong><br />
postemergence programs can provide optimum growth <strong>and</strong> yield (Faircloth,<br />
Patterson, Foshee, Nesbitt, & Goff, 2007).<br />
The area between tree rows is traditionally maintained in grass sod to facilitate<br />
movement of spray equipment that is used for fungicide <strong>and</strong> insecticide applications<br />
during the growing season. Consequently, this is known as the “sod-strip” method of
IPM IN PECAN PRODUCTION<br />
145<br />
orchard floor management. Maintaining a clean (bare ground) strip in the tree row<br />
also facilitates harvest in the fall since nuts can be blown away from the trees into<br />
the sod strips for pickup <strong>by</strong> harvesting equipment.<br />
There is also some use of herbicide in subduing unwanted vegetation in the<br />
traffic lanes where equipment runs between the tree rows. If there is a sod middle,<br />
“chemical mowing” with low rates of glyphosate is a common practice to reduce<br />
excess growth <strong>and</strong> reduce the need to mow (Alabama Cooperative Extension<br />
System, 2007; Ge<strong>org</strong>ia Cooperative Extension Service, 2007). Low rates of<br />
glyphosate are also applied just prior to harvest to reduce regrowth that might<br />
interfere with harvest, as mowing once nuts are on the ground is no longer an option.<br />
A recent practice has been the use of rolling wiper applicators with glyphosate to<br />
remove tall weeds from low-growing desirable plants like “Durana” white clover.<br />
Table 3. Yields of pecans were significantly influenced <strong>by</strong> weed control in irrigation <strong>and</strong><br />
nonirrigated, Fairhope, Alabama USA (Patterson & Goff, 1993).<br />
Irrigation <strong>and</strong><br />
weed control program<br />
Irrigated<br />
Total weed control w/ herbicides<br />
Disking<br />
Mowing<br />
Grass control w/ selective herbicides<br />
No weed control<br />
Mean value for irrigated trees<br />
LSD (P
146<br />
J.D. DUTCHER ET AL.<br />
without weed control growing in both irrigated <strong>and</strong> not irrigated situations produced<br />
only 18.2 <strong>and</strong> 17.5% of the yield, respectively, that was produced <strong>by</strong> trees where<br />
total weed control was maintained over the first 8 years of growth (Table 3). This<br />
research also shows that mowing around newly planted trees, while controlling<br />
annual broadleaf weeds, allowed perennial grasses like bahiagrass to grow, thus<br />
robbing the young trees of fertilizer <strong>and</strong> moisture. Trees in the study that were<br />
mowed only as a means of managing the orchard floor produced 35.6 <strong>and</strong> 21.4% of<br />
the yield (irrigated <strong>and</strong> not irrigated respectively) produced <strong>by</strong> trees where total<br />
weed control was maintained using registered herbicides. This research was<br />
conducted using a treated area of 3 m(dia), centered on the tree row. The 3 m treated<br />
area was arbitrarily selected for this study. Additional research conducted following<br />
this initial study shows that weed-free areas of 3 m(dia) or greater maintained from<br />
planting provided optimum growth <strong>and</strong> yield while areas of 1.8 m (dia) or less<br />
reduced growth <strong>and</strong> eventual yield in the first 2 years of nut bearing (Patterson et al.,<br />
1990). Although the significant <strong>and</strong> detrimental impact of weeds on pecan growth<br />
<strong>and</strong> yield has been documented, weeds can also serve as a host for insect pests<br />
(Norris & Kogan, 2005), <strong>and</strong> negatively influence concentrations of nutrients in<br />
young pecan trees (Goff, Patterson, & West, 1991).<br />
3. BENEFITS OF CRIMSON CLOVER AND LEGUMES USE IN PECAN<br />
ORCHARDS<br />
In the last 30 years, growers have started an integrated approach to weed control <strong>by</strong><br />
seeding the orchard with various cool season legumes. These are grown as<br />
intercrops in the mowed strip or as cover crops over the entire orchard floor. The<br />
intercrop <strong>and</strong> cover crop plants supply nitrogen, suppress weeds, improve the soil,<br />
enhance beneficial insects <strong>and</strong> benefit wildlife. For centuries, legumes have been<br />
used to enhance the fertility <strong>and</strong> structure of agricultural soils. Historical references<br />
as far back as the Roman Empire refer to the benefits these plants can provide. Cato<br />
the Elder (234–149 B.C.) suggested improvements to poor vineyard l<strong>and</strong> <strong>by</strong> interplanting<br />
a legume crop. This crop was then turned under before the plants set seed.<br />
The Chinese have also used legumes to maintain soil fertility through centuries of<br />
cultivation. Legume use was introduced to pecan orchard management in the early<br />
twentieth century. Pecan producers quickly realized the benefits of such plants as<br />
blue lupine, vetch, <strong>and</strong> crimson clover as winter cover crops for the orchard.<br />
Proper orchard management occurs at two separate, yet connected levels. The<br />
orchard floor influences the tree crop <strong>and</strong> its management based on the type of<br />
vegetation or lack thereof found in the orchard. An efficient orchard floor cover does<br />
not compete heavily with trees for moisture <strong>and</strong> nutrients <strong>and</strong> is compatible with<br />
orchard insect populations. Weed competition with tree roots is significant<br />
throughout the life of the tree. In a newly planted orchard, weed competition can<br />
significantly reduce young tree survival <strong>and</strong> can stunt tree growth (Patterson, 2005a,<br />
2005b). In the case of the mature orchard, vegetative competition can rob the soil of<br />
water <strong>and</strong> nutrients intended for the crop, reducing tree growth <strong>and</strong> yield, while also<br />
promoting alternate bearing. Pecan orchards generally consist of sod culture on the<br />
orchard floor with a weed-free herbicide strip approximately 2–4 m wide along the
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147<br />
tree row. Row middles are maintained <strong>by</strong> mechanical mowing or <strong>by</strong> chemical<br />
mowing. The mowed sod middle improves wet weather passage for spraying,<br />
harvesting, <strong>and</strong> other orchard operations.<br />
Pecan trees have an extensive root system, consisting of a tap root which can<br />
penetrate as deep as the soil structure <strong>and</strong> water table permit, <strong>and</strong> small feeder roots<br />
located near the soil surface. While the deeper roots are an aid to survival of the tree<br />
in difficult environmental conditions, the feeder roots in the upper 6–18 in. of soil<br />
supply the bulk of the pecan’s nutritional needs <strong>and</strong> come into direct competition<br />
with vegetation on the orchard floor.<br />
Cool season legumes, such as crimson clover, posses a variety of characteristics<br />
that make them compatible with pecan production. Cool season legumes are not<br />
especially competitive with trees for soil moisture until mid to late spring. They also<br />
serve as an effective source of <strong>org</strong>anically bound nitrogen (N). In addition, cool<br />
season legumes stimulate an early increase in beneficial insect populations. The<br />
environmental benefits of cool season legumes make their use an especially<br />
attractive practice. In addition to the benefits mentioned above, legumes can reduce<br />
weed competition, aid in the cycling of nutrients, build soil <strong>org</strong>anic matter, prevent<br />
soil erosion <strong>and</strong> runoff, <strong>and</strong> serve as an effective source of food <strong>and</strong> habitat for a<br />
variety of wildlife species.<br />
3.1. Pecan Nitrogen Use <strong>and</strong> Compatibility with Crimson Clover<br />
Prior to World War II, legumes were commonly used as an orchard floor cover due<br />
to their N-fixing properties. The arrival of cheap fertilizer sources <strong>and</strong> mowed sod<br />
culture in the orchard led to a decline in the use of legumes as a floor cover in later<br />
years (White, Beaty, & Tedders, 1981).<br />
Of all nutrients applied to pecans, N most commonly limits pecan growth <strong>and</strong><br />
orchard profitability. This element has a dominant influence on vegetative growth<br />
<strong>and</strong> crop production. In recent years, the rising cost of fuel, <strong>and</strong> its effect upon<br />
synthetic fertilizer production, has once again led to a need for alternative sources of<br />
N in many orchard operations. Leguminous plants are one very efficient source of<br />
<strong>org</strong>anic N.<br />
All legumes, including crimson clover, utilize soil-dwelling bacteria that convert<br />
nitrogen from the air into a form that can be used <strong>by</strong> plants. This is termed “nitrogen<br />
fixation”. Only particular strains of bacteria provide optimum N production for each<br />
group of legumes. When the roots of a leguminous plant come into contact with the<br />
appropriate bacteria, the root hairs encircle the bacteria to create a nodule which<br />
houses the bacteria. These lumps on the root surface may range in size from a BB to<br />
a kernel of corn.<br />
Perennial legumes “fix” N during any time of active growth, usually peaking at<br />
flowering. With seed formation, N fixation ceases <strong>and</strong> the nodules slough from the<br />
roots. While they are alive, legumes release little to no nitrogen from the soil. As<br />
they die <strong>and</strong> are decomposed <strong>by</strong> soil micro-<strong>org</strong>anisms, the N in the roots, stalks,<br />
leaves, <strong>and</strong> seeds are converted to a form available to other plants.
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Clover <strong>and</strong> other legumes are capable of supplying significant amount of N to<br />
orchard soils. Studies in Oklahoma suggest that a mixture of legumes including<br />
crimson clover, hairy vetch, red clover, <strong>and</strong> white clover planted to the orchard floor<br />
provided over 100 kg of N/ha. In the same study, pecan leaf N concentrations were<br />
maintained above a threshold of 2.25% <strong>by</strong> the above mixture, as well as <strong>by</strong> crimson<br />
clover alone Blue lupine can fix as much as 168 kg of N/ha, while common vetch is<br />
capable of fixing 92 kg of N (Smith, Shiferaw, & Rice, 1996).<br />
Pecans are an “irregular bearing” crop, meaning that they tend to bear heavy<br />
crop loads for 1–2 years, followed <strong>by</strong> very light crop loads, depending upon various<br />
physiological <strong>and</strong> environmental factors. A general rule of thumb for the N<br />
requirement of pecan trees is 4.5 kg of N for every 45.4 kg of expected crop (Wells,<br />
2007). Depending upon the degree of irregular bearing, mature pecan trees in the<br />
Southeastern USs may require from 78.5 to 168.1 kg of N annually for optimum<br />
production.<br />
Nitrogen uptake in the pecan tree is driven <strong>by</strong> dem<strong>and</strong>. There are two critical<br />
periods of nitrogen dem<strong>and</strong> during the season the first at early foliage growth <strong>and</strong><br />
the second at kernel filling. The early spring foliage flush is nourished primarily<br />
from reserves held within the tree, while the nitrogen dem<strong>and</strong> during the kernel fill<br />
stage is usually satisfied from soil uptake. If N is limited at kernel filling, then the<br />
tree will mobilize N from the foliage to the kernels.<br />
Studies have suggested that crimson clover over-winters dependably in the<br />
southeastern US <strong>and</strong> much of the US pecan belt. A vigorous st<strong>and</strong> of crimson clover<br />
will contribute between 78.5 <strong>and</strong> 168.1 kg of N/ha. When aided <strong>by</strong> moisture <strong>and</strong><br />
warm weather to speed up decomposition, up to half the N available from legumes<br />
can be released within 7–8 weeks. In the light crop or “off” years, the N supplied <strong>by</strong><br />
the clover alone, would be adequate for optimum production. Heavy crop or “on”<br />
years may require low supplemental N rates in order to bring marketable nuts to<br />
maturity <strong>and</strong> provide a return crop the following year.<br />
3.2. Enhancement of Pest Management<br />
Conserving <strong>and</strong> encouraging beneficial <strong>org</strong>anisms is key to achieving sustainable<br />
pest management. The deep red blossoms of crimson clover attract various species<br />
of bees, which feed readily on the abundant nectar. In addition, blooms may harbor<br />
beneficial insects such as the minute pirate bug. Pea aphids <strong>and</strong> blue alfalfa aphids<br />
are commonly associated with crimson clover. Although these species are not pests<br />
of pecan, they serve as alternative food sources for beneficial predators such as<br />
ladybeetles, green lacewings, soldier beetles, predaceous stink bugs, damsel bugs,<br />
<strong>and</strong> hover flies. As the clover declines with the onset of warm weather in June, these<br />
beneficial insects move into the trees to feed on pecan aphids <strong>and</strong> other insect pests,<br />
reducing the need for insecticide application.<br />
In addition to reducing insecticide inputs through enhancing beneficial insect<br />
populations, the use of legumes in the orchard can also reduce herbicide use. As<br />
crimson clover grows, it forms a thick, living mulch. This helps to smother <strong>and</strong><br />
shade out more troublesome, competitive weed species.
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3.3. Soil Building <strong>and</strong> Sustainability<br />
Clover can improve orchard soils in a number of ways. Protection against erosion is<br />
the most obvious benefit, but providing <strong>org</strong>anic matter is an equally important, <strong>and</strong><br />
more long term goal. Clover can provide habitat <strong>and</strong>/or food source for important<br />
soil <strong>org</strong>anisms, break up compacted soil layers, <strong>and</strong> help dry out wet soils.<br />
Erosion deprives orchards of topsoil, the most fertile portion of soil with the<br />
highest amount of <strong>org</strong>anic matter. When soil particles are dislodged <strong>by</strong> rainfall, they<br />
are more vulnerable to runoff. Cool season legumes can reduce the impact of rainfall<br />
on bare ground, slow the action of moving water, increase the soil’s ability to absorb<br />
<strong>and</strong> hold water, <strong>and</strong> help stabilize soil particles. Crimson clover produces more dry<br />
matter (6,237–6,683 kg/ha) than many other legumes <strong>and</strong> is recommended for soil<br />
erosion control because of its high early autumn dry matter production.<br />
Grass/crimson clover mixtures combine fibrous surface roots with long tap roots <strong>and</strong><br />
have been observed to reduce herbicide runoff <strong>by</strong> 94–100%.<br />
As the soil–plant–atmosphere continuum cycles plant nutrients, some are<br />
recovered via plant uptake, some are incorporated into <strong>org</strong>anic matter, some are<br />
adsorbed to mineral <strong>and</strong> <strong>org</strong>anic surfaces, <strong>and</strong> some are precipitated as solid<br />
minerals. Excess nutrients are “lost” or removed from the field <strong>by</strong> runoff or<br />
subsurface flow, potentially ending up in water supplies. Nutrients such as N, that<br />
are the most water soluble <strong>and</strong> mobile in the soil, have the greatest potential for the<br />
pollution of ground <strong>and</strong> surface water (Havlin, Beaton, Tisdale, & Nelson, 2005).<br />
Over-fertilization is common in orchard crops because most growers rely on<br />
synthetic fertilizers. The amount of nitrogen removed <strong>by</strong> the crop in proportion to<br />
that applied is often far less with tree crops than with more traditional crops.<br />
Therefore, the leaching of nitrates into groundwater may be especially serious in<br />
orchard crops (Weinbaum, Johnson, & Dejong, 1992). Wiedenfeld, Fenn,<br />
Miyamoto, Swietlik, <strong>and</strong> Marlene (1999) suggested that sod alone on the orchard<br />
floor does not sufficiently reduce nitrate leaching. Green manures like cool-season<br />
legumes reduce the need for N application <strong>and</strong> aid in nutrient conservation <strong>by</strong><br />
utilizing excess fertilizer not assimilated <strong>by</strong> the pecan trees, preventing undesirable<br />
nutrient levels in streams or lakes.<br />
Winter cover crops such as crimson clover grow primarily during a period of<br />
tree dormancy, when N uptake <strong>by</strong> the crop is at a minimum <strong>and</strong> percolation from<br />
rainfall is often the greatest. Although pecan growers have historically had little<br />
economic incentive to grow cool season legumes solely to prevent nitrate leaching,<br />
it is one of the many benefits they provide.<br />
Orchard floor covers can affect nitrogen uptake <strong>by</strong> the main tree crop if C:N<br />
ratios for the floor cover are high. In such cases, the micro-<strong>org</strong>anisms responsible<br />
for decomposition of the highly carbonaceous plant matter require nitrogen to do so,<br />
<strong>and</strong> can lead to the unavailability of N for the main crop (Brady, 1974). Residue<br />
from a grass/legume mix has a higher C:N ratio than the legume alone. However,<br />
under humid conditions, the C:N ratio of such a mix is less than sod alone. In fact,<br />
ratios for the grass/legume mix are such that the release of N is slow, a scenario in<br />
which many perennial tree crops perform well. Slow release of nutrients also causes<br />
nutrients in the orchard soil to be less vulnerable to loss.
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Soil <strong>org</strong>anic matter is composed of partially decayed <strong>and</strong> partially synthesized<br />
plant <strong>and</strong> animal residues. Although, the <strong>org</strong>anic matter content of a mineral soil is<br />
generally only about 3–5%, its influence on soil properties <strong>and</strong> plant growth are<br />
great.<br />
Due to the work of soil micro-<strong>org</strong>anisms, <strong>org</strong>anic matter should be constantly<br />
renewed <strong>by</strong> the addition of plant residues. Legumes such as crimson clover break<br />
down quickly; however their root systems remain tough <strong>and</strong> fibrous, contributing to<br />
the accumulation of <strong>org</strong>anic matter. The addition of <strong>org</strong>anic matter to soils improves<br />
soil structure, increases water holding capacity, increases cation exchange capacity<br />
(the ability of the soil to act as a short term storage bank for positively charged plant<br />
nutrients), <strong>and</strong> provides more efficient storage of nutrients.<br />
Organic matter functions as a “granulator” of soil mineral particles. In most<br />
cases, the higher the soil <strong>org</strong>anic matter, the more loose, easily managed, <strong>and</strong><br />
productive the soil. Organic matter can also serve as a partial source of N, P <strong>and</strong> S.<br />
Through its effect on the physical condition of the soil, <strong>org</strong>anic matter can increase<br />
the ability of the soil to hold moisture <strong>and</strong> make soil water more available for plant<br />
growth.<br />
Cation exchange is one of the most common <strong>and</strong> important of soil reactions.<br />
The cation exchange capacity (CEC) of a soil represents the capacity of the soil to<br />
hold cation, or positively-charged nutrients such as Ca +2 , Mg +2 , K + , <strong>and</strong> NH 4 + . The<br />
CEC is determined <strong>by</strong> the amount of clay or <strong>org</strong>anic matter present in the soil. Soils<br />
with a higher clay <strong>and</strong> <strong>org</strong>anic matter content have a higher cation exchange<br />
capacity than s<strong>and</strong>y, low <strong>org</strong>anic matter soils. Hydrogen ions from the root hairs <strong>and</strong><br />
soil micro<strong>org</strong>anisms replace nutrient cations from the exchange complex. These<br />
nutrient cations are then forced into the soil solution, where they can be more readily<br />
assimilated <strong>by</strong> the root surface (Brady, 1974). Due to their effects on improving soil<br />
<strong>org</strong>anic matter, legumes can aid in this process.<br />
Legumes help to increase the total number <strong>and</strong> diversity of soil <strong>org</strong>anisms,<br />
which is the key to a healthy, well functioning soil. As <strong>org</strong>anic matter increases,<br />
especially if succulent <strong>and</strong> subject to relatively rapid decay, it encourages microbial<br />
action of the heterotrophic <strong>org</strong>anisms responsible for basic decomposition, as well as<br />
“free-living” bacteria, such as Azobacter, which can also fix N from the atmosphere.<br />
Legumes are closely associated with beneficial fungi, the mycorrhizae, which<br />
produce a water-insoluble protein known as glomalin, which binds <strong>and</strong> glues<br />
together particles of <strong>org</strong>anic matter, plant cells, bacteria, <strong>and</strong> other fungi.<br />
Well aggregated soils are less prone to compaction. Heavy farm implements<br />
such as tractors, sprayers, mowers, shakers, <strong>and</strong> harvesters often make numerous<br />
passes over the orchard floor in a given season. Mycorrhizal fungi also have an<br />
efficient method of absorbing phosphorous (P) from the soil, which they pass on to<br />
their host. Without this relationship, P builds up in the soil. Although it is not<br />
leached, it can runoff into streams <strong>and</strong> rivers through soil erosion. The filaments of<br />
the mycorrhizal fungi effectively extend the root system <strong>and</strong> help the plants tap<br />
more P from the soil. Keeping P in an <strong>org</strong>anic form is the most efficient way to keep<br />
it cycling in the soil.<br />
The culture of cool-season legume crops has both soil <strong>and</strong> nutrient conserving<br />
properties that are highly advantageous <strong>and</strong> readily applicable under most humid
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151<br />
climatic conditions. In areas of low rainfall, the benefits of legumes will be limited.<br />
In such areas decomposition of the crop <strong>and</strong> its nutrient release may be too slow.<br />
Additionally, in such areas, moisture conservation is the primary factor governing<br />
soil <strong>and</strong> crop management. Thus, moisture should be conserved for the main crop.<br />
The residual effects of managing legumes as a cool-season cover crop in the orchard<br />
are also expected to be reduced on excessively s<strong>and</strong>y soils.<br />
3.4. Wildlife Benefits<br />
Due to the limited availability of suitable nesting areas in the United States for earlysuccessional<br />
songbirds, converting a common attribute of the southern agricultural<br />
l<strong>and</strong>scape, such as pecan orchards, to a resource for food <strong>and</strong> reproductive habitat<br />
would provide some of the factors necessary to increase survival <strong>and</strong> nesting<br />
success. Increased abundance of birds <strong>and</strong> beneficial arthropods <strong>and</strong> higher species<br />
richness in agricultural fields have been linked to habitat heterogeneity (Freemark &<br />
Kirk, 2001).<br />
The sod/clover orchard floor mixture along with the pecan overstory allows for<br />
an increased l<strong>and</strong>scape heterogeneity. Birds benefit from an increase in prey, an<br />
increase in cover for nesting sites <strong>and</strong> fledgelings, <strong>and</strong> a reduction in nest loss due to<br />
the elimination of mowing during the nesting season (Best, Whitmore, & Booth,<br />
1990; Rodenhouse, Best, O’Connor, & Bollinger, 1993). In addition to enhancing<br />
the l<strong>and</strong>scape for non-game songbirds, as well as bobwhite quail, wild turkey, <strong>and</strong><br />
mourning dove, cool-season legumes provide high quality forage for whitetail deer<br />
during the late winter when other food sources have dwindled (Rodenhouse, Best,<br />
O’Connor, & Bollinger, 1995).<br />
Clover has been shown to be highly effective at attracting high avian <strong>and</strong><br />
arthropod densities, increasing wildlife <strong>and</strong> agronomic benefits compared with<br />
conventional management of agricultural systems (Cedarbaum, Carroll, & Cooper,<br />
2004; Warburton & Klimstra, 1984). The reduction of input in the clover system,<br />
coupled with its agricultural <strong>and</strong> environmental benefits, makes this system both a<br />
good choice for reducing negative impacts on wildlife <strong>and</strong> surrounding ecosystems,<br />
<strong>and</strong> for reducing input costs.<br />
3.5. Establishment <strong>and</strong> Maintenance<br />
In order to establish an adequate st<strong>and</strong>, crimson clover should be drilled at 16.7–20<br />
kg/ha or broadcast at 22.4–3.6 kg/ha. Establishment should be completed as soon as<br />
possible following pecan harvest, preferably in November–December. If clover is<br />
seeded prior to harvest, many seeds are removed from the orchard floor with the<br />
sweeping <strong>and</strong> harvesting process. Since legumes require the presence of rhizobial<br />
bacteria to effectively fix N, it is important to obtain the correct rhizobial inoculant<br />
for the legume being grown. Fresh inoculant <strong>and</strong> a sticking agent should be mixed<br />
with the seed. Otherwise, there will be few nodules <strong>and</strong> N fixation will be low. Soil<br />
pH should be maintained at 6.5 because Rhizobia bacteria cannot function properly<br />
under highly acidic conditions <strong>and</strong> will die in soils with pH below 5.0.
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Many southeastern orchards have well established populations of annual<br />
ryegrass. Where this occurs, the ryegrass often competes with <strong>and</strong> inhibits growth of<br />
clover. This can be prevented <strong>by</strong> the application of a low rate (1.12 kg/ha) of<br />
sethoxydim herbicide in February. The rye grass does not have to be eliminated,<br />
only stunted <strong>by</strong> this application in order to release clover from this competition.<br />
By foregoing mowing of the orchard until clover has gone to seed, producers can<br />
take advantage of crimson clover’s excellent natural re-seeding ability. This will allow<br />
a period of 3–5 years before clover will need to be re-seeded <strong>by</strong> the grower. S<strong>and</strong>y<br />
sites will need to be re-seeded sooner than loamy or clay soils, therefore soil type<br />
should be taken into consideration when estimating the need for re-establishment.<br />
3.6. Costs <strong>and</strong> Savings<br />
The approximate cost of crimson clover seed <strong>and</strong> bacterial inoculum required to<br />
produce N-fixing nodules is approximately $99/ha. At 2005 N prices of $178/ha,<br />
this represents a difference of $79/ha. Clover can replace from 50 to 100% of<br />
synthetic N applied to pecan orchards, depending on the pecan crop load in a given<br />
year. This would save growers approximately $89–178/ha <strong>and</strong> significantly reduce<br />
the grower’s reliance on synthetic N. Reduced maintenance <strong>and</strong> mowing compared<br />
to grass covers creates further economic savings <strong>and</strong> reduces fuel consumption.<br />
Pecan acreage is widely dispersed <strong>and</strong> hard to track, but reliable estimates<br />
indicate that pecans are grown on approximately 550,000 acres in the US, with<br />
Ge<strong>org</strong>ia making up about ¼ of the total USA acreage. This would indicate a<br />
potential savings of approximately $19,800,000–39,600,000 in N costs, as well as a<br />
41,250 t reduction in the use of synthetic N nationwide with the use of N-fixing<br />
legume culture applied to orchard floor management.<br />
One of farming’s greatest challenges is to keep N in a stable, storable form<br />
until needed <strong>by</strong> the crop. The use of <strong>org</strong>anic N, such as that produced <strong>by</strong> legumes, is<br />
an ideal way to accomplish this. Combining warm season sod culture <strong>and</strong> cool<br />
season legumes is a practical <strong>and</strong> effective strategy for conserving <strong>and</strong> supplying<br />
nitrogen for orchard crops, as well as enhancing stewardship of the environment<br />
through the enhancement of soil sustainability, beneficial insects, weed suppression,<br />
<strong>and</strong> wildlife.<br />
4. INTEGRATED PEST MANAGEMENT IN PECAN ORCHARDS<br />
Research indicates that biological control is effective with introduced biological<br />
control agents against pecan aphids (Tedders, Weaver, & Wehunt, 1973; Tedders,<br />
Reilly, Wood, Morrison, & Lofgren, 1990; Tedders & Schaefer, 1994; Mizell,<br />
1984), pecan weevil (Dutcher & Sheppard, 1983; Shapiro-Ilan, 2001; Shapiro-Ilan,<br />
Cottrell, & Gardner, 2004)), <strong>and</strong> pecan leaf scorch mite (Dutcher et al., 2006). Two<br />
biological controls that have been readily adopted <strong>by</strong> pecan growers are the<br />
enhancement of aphidophagous insects with orchard floor management <strong>and</strong><br />
reductions in pecan weevil sprays.
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153<br />
Orchard floor management techniques may improve biological control of<br />
pecan aphids. In improved orchards, tree density typically ranges from 12 to 60 trees<br />
per hectare. An orchard floor with mowed sod <strong>and</strong> herbicide strips in tree rows is<br />
excellent for harvesting the nuts but has low vegetational diversity (Dutcher, 1993).<br />
Natural enemies of aphids <strong>and</strong> other pecan insect pests are more abundant when the<br />
orchard floor is sown with plants that provide alternate prey, nectar, <strong>and</strong> pollen<br />
when pest populations are low. Orchards may require 15–30 trips <strong>by</strong> heavy<br />
machinery each year for all production <strong>and</strong> harvesting operations, leading to soil<br />
compaction (Bugg, Sarrantonio, Dutcher, & Phatak, 1991). Mowing can be reduced<br />
substantially <strong>by</strong> replacing turf grasses with clover (Rice, 1994). Previous studies<br />
have shown increased diversity <strong>and</strong> abundance of native aphid-feeding insects<br />
(aphidophaga) with alternative groundcover management in pecan Rice et al. (1998)<br />
found clover plus vetch to harbor significantly larger populations of ladybeetles<br />
(Family: Coccinellidae) than turf grass cover. Significantly higher populations of<br />
ladybeetles were found in various cool (Bugg, Dutcher, & McNeill, 1990) <strong>and</strong><br />
warm-season (Bugg & Dutcher, 1989) covers. Unfortunately in both cases biological<br />
control of pecan aphids did not increase significantly. Multicolored Asian<br />
ladybeetle, Harmonia axyridis (Pallas), has been successfully introduced <strong>and</strong><br />
established into the pecan belt since the above experiments were conducted.<br />
Multicolored Asian ladybeetle is a much more effective predator on pecan aphids<br />
than native ladybeetles. Even though Rice et al. (1998) did not find a significant<br />
increase in biological control overall in groundcover-enhanced orchards, they did<br />
observe an increase in one isolated orchard where multicolored Asian ladybeetle had<br />
recently become established.<br />
Culturing ladybeetles on alternate prey aphids on crapemyrtle plants grown on<br />
the orchard floor until pecan aphids become more abundant may be effective (Mizell<br />
& Knox, 1993). Crapemyrtle aphids is a good c<strong>and</strong>idate as an alternate prey for<br />
aphidophaga in the pecan system because they peak on crapemyrtle plants about 2<br />
weeks before pecan aphids. This is ideal timing to build up aphidophaga before the<br />
expected peak in pecan aphids. In addition, crapemyrtle aphid <strong>and</strong> black pecan aphid<br />
are taxonomically similar <strong>and</strong> are attacked <strong>by</strong> the same natural enemies (Mizell &<br />
Schiffhauer, 1987). Intercrops sown away from the herbicide strip <strong>and</strong> in the mowed<br />
sod compete with grasses <strong>and</strong> not the trees <strong>and</strong> have additional benefits. Combinations<br />
of red <strong>and</strong> white clovers or clover plus vetch provide adequate nitrogen for pecan<br />
(Smith et al., 1996; Diver & Ames, 2000). Supplemental nitrogen fertilizer is effective<br />
in maintaining leaf nitrogen concentration at a healthy level when it is applied to the<br />
herbicide strip or through the irrigation system (Worley, 1994).<br />
Native <strong>and</strong> introduced natural enemies of the black pecan aphids do not reduce<br />
aphid populations with sufficient speed to prevent serious damage. The population<br />
dynamics are well understood (Kaakeh & Dutcher, 1992). Early warning scouting<br />
techniques are used to measure abundance, population distribution, <strong>and</strong> predict<br />
outbreaks (Dutcher & Kaakeh, 1992). Black pecan aphid feeding leads quickly to<br />
leaflet abscission (Wood, Tedders, & Thompson, 1985; Tedders & Wood, 1985;<br />
Tedders, 1978), <strong>and</strong> control is achieved <strong>by</strong> quickly resorting to chemical control<br />
whenever black pecan aphid abundance exceeds one aphid per compound leaf<br />
(Dutcher, 1983; Dutcher & Htay, 1985).
154<br />
J.D. DUTCHER ET AL.<br />
Secondary predators interact with biological controls <strong>and</strong> these can enhance or<br />
hinder control effectiveness. For example, insects are a major source of nutrition for<br />
red imported fire ants, Solenopsis invicta Buren (Hymenoptera: Formicidae). These<br />
ants are important predators of pests including southern green stink bug (Krispyn &<br />
Todd, 1982), cowpea curculio (Russell, 1981) <strong>and</strong> pecan weevil (Dutcher &<br />
Sheppard, 1983). Pecan weevil larval populations are consistently reduced <strong>by</strong> 33%<br />
after the larvae drop to the soil surface from the pecans <strong>and</strong> before they burrow into<br />
the ground (Dutcher & Sheppard, 1983). Red imported fire ants also interact with<br />
aphids <strong>and</strong> aphidophaga in the pecan trees (Tedders et al., 1990). Ant foraging can<br />
be partitioned with insecticide barriers sprayed on the tree trunks so that red<br />
imported fire ants will remain on the soil surface to prey on weevils <strong>and</strong> not interfere<br />
with aphidophagous insects in the trees (Dutcher, Estes, & Dutcher, 1999). The<br />
effect of these trunk sprays has been effective (Dutcher, 2004; Dutcher et al., 1999)<br />
<strong>and</strong> ineffective in reducing aphid populations (Harris et al., 2003). Red imported fire<br />
ants can tunnel under the insecticide barrier without becoming intoxicated <strong>and</strong><br />
produce a trail to the tree crown, esp. on older trees with heavy bark. Farnesol, an<br />
ant repellent that form an impassable odor plume around the trunk successfully<br />
prevents Argentine ants from foraging in citrus trees (Shorey, Gaston, Gerber, Sisk,<br />
& Phillips, 1996). Current research has found that farnesol was not an effective<br />
repellent of ants on pecan trees but certain plant extracts (neem extract, sesbania<br />
extract), natural compounds (methyl anthranilate, methyl myristate) <strong>and</strong> an<br />
industrial repellent (methyl carbitol) are effective ant repellents that prevent foraging<br />
in pecan trees (Dutcher & Beaver, 2005).<br />
Pecan weevil has a relatively long life cycle <strong>and</strong> lower reproductive capacity in<br />
comparison to other pecan insect <strong>and</strong> mite pests (Table 2). Growers may achieve<br />
control <strong>by</strong> integrating chemical control for adults biological control with soil<br />
application entomopathogens <strong>and</strong> entomophillic nematodes, <strong>and</strong> red imported fire<br />
ants with <strong>and</strong> removal of alternate host trees from the woodlots adjacent to the<br />
orchard to reduce immigration of adults into the orchard. Risk rating (Mizell, 1984)<br />
estimates the relative probability of pest outbreak based on all pertinent information<br />
that is known about a particular area <strong>and</strong> may be useful in integrating control<br />
methods for pecan weevil. Pecan cultivars <strong>and</strong> trees of different ages (sizes) differ<br />
considerably to the susceptibility to injury <strong>by</strong> pecan weevil (Worley & Mullinix,<br />
1997). Certain pecan cultivars have a narrow window of susceptibility to pecan weevil<br />
oviposition with either a short kernel development time, or an early or late onset of<br />
kernel development (Harris, 1985). Weevil can be controlled in these cultivars with 2–3<br />
applications of carbaryl compared to 4–5 applications for st<strong>and</strong>ard cultivars.<br />
Precision applications of carbaryl to tree trunks <strong>and</strong> spot treatments in highly<br />
infested portions of the orchard stems may reduce nut damage in the pecan tree. Nut<br />
damage is higher in trees with higher densities of weevils emerging from the soil<br />
directly beneath the tree (Dutcher et al., 2003). In early replicated field trials, trunk<br />
sprays effectively killed adult weevils on the trunk for up 13 days after application of<br />
carbaryl (Cottrell & Wood, 2003). It has been estimated that 70–80% of the adult<br />
weevils fly to the trunk first (Raney & Eikenbary, 1968) <strong>and</strong> could thus be targeted for<br />
insecticide application to manage pecan weevils. This would reduce entire canopy<br />
sprays, which are known to be detrimental to natural enemies <strong>and</strong> flare aphid <strong>and</strong> mite
IPM IN PECAN PRODUCTION<br />
155<br />
populations (Dutcher & Payne, 1983). The trees in native groves have a unique nut<br />
phenology in each tree adding to the variability in pecan weevil distribution (Reid &<br />
Mulder, 2003). Pecan weevil distribution in the orchard can be estimated from tree-totree<br />
measurements of % nut damage, crop load, <strong>and</strong> known population parameters of<br />
the weevil (Harris, 1985) <strong>and</strong> then validated <strong>by</strong> extensive trapping of emerging adults<br />
with cone emergence traps from a known area of the soil surface (Raney, Eikenbary,<br />
& Flora, 1970). Accurate weevil distribution maps would allow the precision<br />
application of soil applied biocontrol agents <strong>and</strong> foliage <strong>and</strong> trunk sprays of carbaryl.<br />
Significant risk of hemipteran kernel damage is associated with soybean<br />
plantings (<strong>and</strong> other alternate host plants) adjacent to the pecan orchards <strong>and</strong> the<br />
lack of a trap crop for monitoring <strong>and</strong> control of the hemipterans. Spot treatments of<br />
insecticide sprays to the trees in the first two border rows adjacent to the alternate<br />
host plants are effective in reducing stink bug damage (kernel spot) throughout the<br />
orchard. Legume trap crops between the trees <strong>and</strong> the alternate host plants are<br />
effective <strong>and</strong> have been used <strong>by</strong> pecan growers for reducing kernel spot. Even low<br />
black aphid populations on less susceptible cultivars cause significant leaf damage<br />
<strong>and</strong> defoliation. However, on less susceptible cultivars the onset of the outbreak is<br />
often several weeks later than on susceptible cultivars (Wood & Reilly, 1998).<br />
Kernel spot is caused <strong>by</strong> several species of true bugs belonging to the families,<br />
Pentatomidae <strong>and</strong> Coreidae. Initially, kernel spot was thought to be caused <strong>by</strong><br />
disease <strong>and</strong> treated as such until it was proven (Adair, 1927) that these conditions<br />
were caused <strong>by</strong> several species of kernel feeding hemipterans. The primary kernel<br />
feeding hemipteran pests of pecan include the southern green stink bug, Nezara<br />
viridula; green stink bug, Acrosternum hilare; brown stink bug, Euschistus servus;<br />
Dusky stink bug, Euschistus tristigmus <strong>and</strong> the leaffooted bugs, Leptoglossus<br />
phyllopus <strong>and</strong> L. oppositus. All of these insects are phytophagus <strong>and</strong> feed on a wide<br />
range of plants (McPherson & McPherson, 2000). Stinkbugs find crops such as<br />
cowpeas <strong>and</strong> soybeans more appealing than pecan trees when plots of these crops<br />
are planted near pecan orchards, gravitating toward the trap crop <strong>and</strong> away from the<br />
trees.<br />
The primary challenges pecan producers face in managing these pests include<br />
the lack of economic thresholds to make management decisions, the long period of<br />
susceptibility to damage (nut set to harvest), the difficulty in scouting for damaging<br />
populations <strong>and</strong> the limitations on insecticide use near harvest. Leguminous trap<br />
crops, sown adjacent to seedling <strong>and</strong> improved pecan orchards, effectively <strong>and</strong><br />
consistently reduce the incidence of kernel spot <strong>by</strong> 50% in improved pecan orchards<br />
(Smith, 1996, 1999). The trap crops are sprayed as the pods mature with an<br />
insecticide to kill the hemipterans before they enter the orchard (Coolman, 2003).<br />
Growing trap crops is beneficial for owners of small pecan orchards, as well as<br />
people who want to grow their pecan crops <strong>org</strong>anically. Growing a trap crop around<br />
the orchard controls stink bugs without spraying the trees. Sunflower, s<strong>org</strong>hum <strong>and</strong><br />
millet are also attractive to kernel-feeding hemipterans <strong>and</strong> produce seed that is<br />
attractive to hemipterans in the early fall at the same time as the pecans are<br />
susceptible to kernel spot. In native pecan groves, trap crops or broad scale<br />
application of pesticides to control stink bugs populations are not practical since<br />
livestock <strong>and</strong> poultry are part of the system. The mid-summer weeds in the groves
156<br />
J.D. DUTCHER ET AL.<br />
are attractive to kernel-feeding hemipterans <strong>and</strong> the weeds provide a place for stink<br />
bug populations to develop within the grove itself <strong>and</strong> mowing of these weeds is an<br />
alternative control technique. Trap crops also provide excellent food for quail. Many<br />
pecan growers already plant small grains near the orchard border in the fall to feed<br />
wildlife <strong>and</strong> improve hunting, esp. for quail. A pecan grower in Texas achieved<br />
significant reductions in the incidence of kernel spot <strong>by</strong> plant a nontreated trap crop<br />
of black-eyed peas (United States Environmental Protection Agency, 2004).<br />
Integrated pest management came to the forefront in pecan pest control after<br />
problems arose with pest resurgence, pesticide resistance, pest replacement, <strong>and</strong> an<br />
increase in virulence of the pecan scab fungus. These problems lead to outbreaks of<br />
aphids, mites, leafminers <strong>and</strong> pecan scab. Growers, researchers <strong>and</strong> extension<br />
specialists developed <strong>and</strong> implemented integrated pest management methods in<br />
attempts to solve many of these problems. Current pest management practices for<br />
pecan orchards are a genuine integration of various natural, cultural, biological <strong>and</strong><br />
chemical control techniques. These include: monitoring crop load, orchard floor<br />
management, soil amendments, scouting pest populations, enhancement of on<br />
natural enemies, decision models, action thresholds, looking for pecan scab<br />
resistance in pecan cultivars, inoculative release of introduced insect <strong>and</strong> mite<br />
predators, planting intercrops, selective timing of chemical pesticide sprays <strong>and</strong><br />
selective pesticides. Reducing broad spectrum insecticide spray frequency with<br />
improved monitoring techniques, weather models <strong>and</strong> assessments damage impact<br />
coupled with spot treatments has reduced the incidence of secondary pest resurgence<br />
after treatments for pecan weevil <strong>and</strong> kernel feeding hemipterans (Dutcher & Payne,<br />
1983). Biological controls <strong>and</strong> biorational or selective insecticides are under<br />
development for other insect <strong>and</strong> mite problems are effectively controlled with<br />
(Dutcher et al., 2003).<br />
Integrated pest management research <strong>and</strong> extension work (Dutcher et al., 2003)<br />
in the past 25 years has developed new methods that reduce the amount of insecticide<br />
used <strong>by</strong> 35% (Smith et al., 2002). The future of pecan integrated pest management lays<br />
in the development of reduced fungicide spray frequency in the southeastern USA<br />
during time periods of low humidity <strong>and</strong> leaf wetness <strong>and</strong> reduced soil compaction <strong>and</strong><br />
herbicide use through orchard floor management. Integration of the tactics enhances<br />
aphidophagous insects, improves the soil, <strong>and</strong> reduces the production costs for the<br />
pecan grower. Above <strong>and</strong> beyond these improvements, integrated pest management in<br />
the pecan orchard is the only known strategy for avoidance of secondary pest<br />
resurgence, replacement of a primary pests, <strong>and</strong> pesticide resistance development.<br />
These phenomena can double the costs of pest control.<br />
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7<br />
LOCUST HABITAT MONITORING AND RISK<br />
ASSESSMENT USING REMOTE SENSING AND GIS<br />
TECHNOLOGIES<br />
ALEXANDRE V. LATCHININSKY 1 AND RAMESH<br />
SIVANPILLAI 2<br />
1 Department of Renewable Resources, University of Wyoming,<br />
Laramie, WY 82071, USA<br />
2 Department of Botany <strong>and</strong> Wyoming<br />
Geographic Information Science Center, University of Wyoming,<br />
Laramie, WY 82071, USA<br />
Abstract. Locust outbreaks occur on all continents except Antarctica <strong>and</strong> can affect the livelihoods of one<br />
in 10 people on Earth. To prevent economic <strong>and</strong> environmental losses, locust breeding areas should be<br />
periodically monitored, <strong>and</strong> an early detection-early response strategy should be in place. Traditional,<br />
ground survey methods are inefficient to adequately address the large spatial scale of the locust problem.<br />
Remote Sensing <strong>and</strong> the associated geospatial technologies can provide timely data to assess the risk of<br />
impending locust outbreaks. This information could be used for targeted preventive management actions<br />
in the locust breeding areas. Remotely sensed data are used for monitoring habitats of certain species such<br />
as the Desert, Migratory <strong>and</strong> Australian Plague locusts. However, the vast potential of this technology<br />
remains untapped for other locusts. This chapter provides a review of remote sensing <strong>and</strong> GIS concepts,<br />
types of data collected <strong>by</strong> various remote sensing satellites, <strong>and</strong> applications of geospatial tools for locust<br />
habitat monitoring <strong>and</strong> risk assessment.<br />
1. INTRODUCTION<br />
Locust outbreaks <strong>and</strong> subsequent destruction of vegetation result in ecological,<br />
environmental <strong>and</strong> economic problems. Locust swarms can devour green vegetation,<br />
including agricultural crops, across large geographic areas there<strong>by</strong> upsetting the<br />
ecological processes (e.g. carbon <strong>and</strong> water cycles) of the region or any l<strong>and</strong>scape.<br />
Rapid loss in vegetation cover can result in soil erosion <strong>and</strong> increased run off. Crop<br />
damages could result in catastrophic losses to farmers, <strong>and</strong> this problem could be<br />
acute for small, subsistence farmers throughout the world <strong>and</strong> especially for those in<br />
developing countries. Furthermore, locust control efforts, which involve large-scale<br />
applications of broad-spectrum insecticides, can produce negative impact on the<br />
environment <strong>and</strong> continue to be very costly, even in the twenty-first century.<br />
163<br />
A. <strong>Ciancio</strong>, K.G. Mukerji (eds.), Integrated Management of Arthropod Pests<br />
<strong>and</strong> Insect Borne Diseases, Integrated Management of Plant Pests <strong>and</strong> Diseases 5,<br />
DOI 10.1007/978-90-481-8606-8_7, © Springer Science+Business Media B.V. 2010
164<br />
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In 2003–2005 a Desert locust outbreak affected 8 million people mostly in<br />
Africa, with estimated damage to crops at 80–100% (Brader et al., 2006). To combat<br />
the outbreak, 13 million ha were treated with neurotoxins in 26 countries. The cost<br />
of the international campaign, including the food aid to affected populations,<br />
amounted to half a billion US dollars (Belayneh, 2005).<br />
In order to protect the farmers <strong>and</strong> the environment from such catastrophes,<br />
several national <strong>and</strong> international agencies <strong>and</strong> <strong>org</strong>anizations are involved in a host<br />
of prevention <strong>and</strong> control activities. These activities are aimed at either minimizing<br />
the large-scale locust plagues or at quickly containing them following an initial<br />
outbreak. Since the geographic area involved is often large (across national<br />
boundaries), coordination is required in the form of information exchange on the<br />
status of locust swarm distribution <strong>and</strong> damage. In most countries information on<br />
locust nymphal development <strong>and</strong> swarm formation is collected through groundbased<br />
surveys. Data collected <strong>by</strong> field surveys are reported to the national locust<br />
control units, which then share them with other national <strong>and</strong> international agencies.<br />
To assess locust risks <strong>and</strong> develop preventive measures data on l<strong>and</strong> cover habitat<br />
condition are required. Vegetation represents the essential component of the locust<br />
habitat, providing the insects with nutrition <strong>and</strong> shelter.<br />
Under the preventive mode, locust control specialists also need information on<br />
elevation (or topography), soil moisture, temperature <strong>and</strong> rainfall, in addition to the<br />
vegetation type, status <strong>and</strong> growth. Specialists use this information to set up<br />
effective surveys to assess locust egg-pod or nymphal distribution. During an<br />
outbreak, near real-time data on vegetation damage, hopper b<strong>and</strong> <strong>and</strong> swarm<br />
movement will be essential for assessing risks <strong>and</strong> prioritizing areas for curative<br />
treatments. Under either circumstances reliable methods are necessary for collecting<br />
information on vegetation status or assessing the damage to the native vegetation or<br />
crops resulting from locust outbreaks. Traditional, ground-based survey methods are<br />
inadequate to provide accurate <strong>and</strong> timely information about an ongoing locust<br />
outbreak <strong>and</strong> devise efficient management approaches, since the locust hopper b<strong>and</strong>s<br />
move several km <strong>and</strong> swarms can travel up to 200 km in a day (Uvarov, 1977).<br />
Remote sensing technology can provide necessary data for assessing locust<br />
outbreak threats <strong>and</strong> post-outbreak damage. Remote sensing technology is a means<br />
to rapidly collect information on vegetation <strong>and</strong> earth surface conditions for<br />
relatively large geographic areas. These data are routinely used for assessing the<br />
status of l<strong>and</strong> <strong>and</strong> natural resources or for assessing the magnitude of events such as<br />
wildfires <strong>and</strong> hurricanes. Satellite images were used extensively to coordinate the<br />
rescue <strong>and</strong> recovery efforts following the tragic devastation of the South Asian<br />
Tsunami in 2004 (Kumar, Chingkhei, & Dolendro, 2007; Wikantika, Sinaga, Hadi,<br />
& Darmawan, 2007). Satellites can download these data rapidly to receiving stations<br />
on the ground enabling the users to visualize the data in near-real time. Currently,<br />
there are remote sensing satellites that collect data for the entire earth every 2 days.<br />
In other words, one can monitor the status of any location on the earth’s surface<br />
every 2 days. Advances in computing hardware <strong>and</strong> software have enabled<br />
sophisticated processing of large volumes of data that was not possible until a few<br />
years ago. Through the use of such data, information on earth surface conditions can<br />
be updated more frequently, in comparison to the traditional survey methods.
LOCUST REMOTE SENSING AND GIS<br />
165<br />
Image data collected <strong>by</strong> the satellites can be incorporated with other types of<br />
information (roads, rivers, villages <strong>and</strong> administrative boundaries) in a geographic<br />
information system (GIS). Using a GIS one could generate a map showing<br />
potential areas of interest that are within a specified distance from major roads.<br />
This information could be used for targeted locust field surveys or to identify the<br />
extent of areas that cannot be easily accessed. Also using the information on<br />
administrative boundaries it is possible to generate summary maps showing the<br />
extent of infestation <strong>and</strong> damage, per administrative unit. Such information could<br />
be generated in the form of both maps <strong>and</strong> reports more easily <strong>and</strong> quickly in<br />
comparison to the traditional cartographic methods. In the US, wildfire maps are<br />
updated daily using satellite data to enable the firefighters to assess the extent <strong>and</strong><br />
direction of the wildfires (Keane, Burgan, & Van Wagtendonk, 2001; Hessburg,<br />
Reynolds, Keane, James, & Salter, 2007). Also, the Food <strong>and</strong> Agriculture<br />
Organization of the United Nations (FAO) uses GIS extensively to map the l<strong>and</strong><br />
conditions in Africa <strong>and</strong> generate monthly Desert locust information bulletins (see<br />
http://www.fao.<strong>org</strong>/ag/locusts/en/info/info/index.html).<br />
However, remote sensing technology is not capable of addressing all the<br />
information needs of the locust control specialists. Its potential is oversold across<br />
several applications resulting in bad reputation among users (Wynne & Carter,<br />
1997). The process of converting data to useful information is rigorous <strong>and</strong> requires<br />
substantial training <strong>and</strong> knowledge on the part of an image analyst. These skills are<br />
critical to successfully extract information off of the images. Nevertheless, several<br />
of these risks could be addressed <strong>by</strong> careful planning <strong>and</strong> adequate training of the<br />
analysts in the use of image processing for information extraction. If implemented<br />
correctly, remotely sensed <strong>and</strong> GIS technologies can provide essential information<br />
for managing locust problems worldwide.<br />
2. REMOTE SENSING, GEOGRAPHIC INFORMATION SYSTEMS (GIS),<br />
AND GLOBAL POSITIONING SYSTEMS (GPS)<br />
2.1. Remote Sensing<br />
Remote sensing is defined as the science <strong>and</strong> art of making observations <strong>and</strong><br />
measurements about objects without coming into physical contact (Campbell, 2006).<br />
For example, a human eye remotely senses or “sees” <strong>by</strong> responding to the radiation<br />
emanating from the surrounding objects without any physical contact. All objects<br />
above absolute zero (0 K or –373°C) emit electromagnetic radiation <strong>and</strong> also interact<br />
with the incoming solar radiation. When solar radiation comes in contact with an<br />
object it can be reflected, transmitted or absorbed to be re-emitted <strong>and</strong> the pattern of<br />
this interaction is unique for each object, which is referred as the spectral signature<br />
for that object. For example, green leaves absorb radiation in the blue <strong>and</strong> red<br />
regions but emit in the green region, hence they appear green to human eyes.<br />
Changes in the leaf chlorophyll content alter the reflectance pattern which results in<br />
different colors of the leaves to human eyes.
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Table 1. Spectral ranges in the electromagnetic spectrum (in nm unless otherwise specified).<br />
Spectral range<br />
Name<br />
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Remote sensing is categorized as passive or active based on the source of the<br />
electromagnetic radiation. In passive remote sensing, sensors record the radiation<br />
emitted or reflected <strong>by</strong> earth surface features. For example, when data are recorded<br />
in the form of images in bright sunlight (or outdoors) without any other source of<br />
radiation it is termed as passive remote sensing. Black & white photos have been in<br />
use for more than a century <strong>and</strong> extensively in World War II to identify <strong>and</strong> destroy<br />
enemy targets. Color infrared photos were acquired since mid-1950s <strong>and</strong> have found<br />
widespread use in vegetation mapping <strong>and</strong> monitoring (Jenson, 2006). Digital<br />
sensors, mounted in satellites, aerial platforms <strong>and</strong> space shuttles, are used more<br />
frequently for collecting remotely sensed data. Digital data are available in ready-touse<br />
formats <strong>and</strong> can be processed more efficiently than hard copy aerial<br />
photographs. Availability of these data in digital format coupled with the advances<br />
in computing technology, have resulted in increased use of remote sensing for<br />
numerous applications.<br />
Active remote sensing systems use their own source of electromagnetic radiation<br />
that is targeted towards various objects <strong>and</strong> records the interacted information that<br />
reaches the sensor. If one uses a flash light in the camera to illuminate indoor objects<br />
for recording images, this is active remote sensing. Examples of active remote<br />
sensing data include RADAR <strong>and</strong> LIDAR images that are acquired <strong>by</strong> targeting<br />
electromagnetic radiation in specific regions on various features <strong>and</strong> recording their<br />
interaction pattern. Active remote sensing technology provides opportunities for<br />
acquiring images during night time or cloudy days. Both RADAR <strong>and</strong> LIDAR can<br />
penetrate through the top of the vegetation canopy, which is not possible in passive<br />
remote sensing, enabling vertical characterization of forests <strong>and</strong> other features.<br />
RADAR can also penetrate soil, hence it is used in archeology for locating <strong>and</strong><br />
mapping large hidden structures <strong>and</strong> artifacts.<br />
Utility of remotely sensed data is influenced <strong>by</strong> its spatial, spectral, temporal <strong>and</strong><br />
radiometric resolutions among others. Spatial resolution determines the size of the<br />
smallest feature that can be identified in an image. No st<strong>and</strong>ard rules exist to<br />
categorize remotely sensed data based on its spatial resolution, however certain<br />
guidelines have evolved over time. Images are categorized as high (
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Table 2. Remote sensing satellites <strong>and</strong> their data characteristics.<br />
Satellite & country Spectral b<strong>and</strong>s Pixel<br />
size (m)<br />
Swath (km)<br />
Coarse resolution<br />
NOAA-GOESS (USA) 1,000 >2,000<br />
SPOT VEG (France) 1,000<br />
TERRA/MODIS (USA) 250 >2,000<br />
500<br />
1,000<br />
Moderate resolution<br />
L<strong>and</strong>sat 5 (USA) B, G, R, 3 IR 30 185<br />
SPOT-2 (France) G, R, 2 IR 20 120<br />
IRS 1C (India) G, R, 2 IR 23 70, 142<br />
IRS 1D G, R, 2 IR 23 70, 142<br />
SPOT-4 G, R, 2IR 20 120<br />
L<strong>and</strong>sat 7 B, G, R, 3IR 30 185<br />
TERRA/ASTER<br />
(Japan/USA)<br />
G, R, IR<br />
4 IR<br />
3 Thermal IR<br />
15<br />
30<br />
90<br />
EO-1 (USA) 30 37<br />
Proba (ESA) 18, 36 14<br />
SPOT-5 10 120<br />
IRS ResourceSat 20 24, 140, 740<br />
IRS-AWiFS (India) 56 350<br />
CBERS-2 (China/Brazil) 20 113<br />
FormaSat (Taiwan) 8 24<br />
ThaiPhat (Thail<strong>and</strong>) 36 600<br />
MONITOR-E-1 (Russia) 20 94, 160<br />
Beijing-1 (China) 32 600<br />
TopSat (UK) 5 10, 15<br />
ALOS (Japan) 10 35, 70<br />
60<br />
Temporal resolution is related to the time lapse between successive image<br />
acquisitions. For example, L<strong>and</strong>sat 5 – TM satellite acquires data every 16th day for<br />
any given location on the surface of the earth, <strong>and</strong> therefore its temporal resolution<br />
is 16 days. Other satellites (e.g., AVHRR) collect data on daily basis.<br />
Radiometric resolution is a measure of precision of the recorded data <strong>and</strong><br />
measured in bits. In an 8-bit data recording device, 256 (2 8 ) levels of brightness<br />
values can be recorded, whereas 10-bit device can record 1024 (2 10 ) levels of<br />
brightness values. Satellite <strong>and</strong> aerial based remotely sensed data are available in<br />
difference combinations of resolutions (example, 30 m spatial, 6 spectral b<strong>and</strong>s, 16<br />
day temporal <strong>and</strong> 8-bit radiometric resolutions) <strong>and</strong> it is up to the analyst to select<br />
the correct type of data for matching the informational needs of a task.
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2.2. Information Extraction<br />
Remotely sensed data are available in digital format (earlier, these images were<br />
printed as hard copy maps <strong>and</strong> features were manually interpreted). Analysts can<br />
display the images in any image processing software (Table 3). Depending on the<br />
specific informational needs, enhancements or classification can be carried out on<br />
these images. Enhancement refers to a set of image processing steps where<br />
information content about one or more features in the image is highlighted.<br />
Enhanced products can be used to prepare hard copy maps or further digital<br />
processing. Vegetation indices are computed from these images for monitoring<br />
vegetation condition. Vegetation indices computed from two different time periods<br />
are useful for change assessment studies.<br />
Table 3. Selected examples of remote sensing software.<br />
Software Manufacturer Website<br />
ENVI ITT VIS www.ittvis.com<br />
ERDAS imagine ERDAS Inc. www.erdas.com<br />
ER mapper ERDAS Inc www.erdas.com/ermapper<br />
IDRISI Clark Labs www.clarklabs.<strong>org</strong><br />
ILWIS ITC www.itc.nl/ilwis<br />
Image analyst Intergraph www.intergraph.com<br />
PCI PCI Geomatics www.pcigeomatics.com<br />
Mapping earth surface features requires a suite of sophisticated image processing<br />
tools, such as unsupervised <strong>and</strong> supervised, neural network <strong>and</strong> fuzzy logic<br />
classifiers. Each algorithm has its own advantage <strong>and</strong> the analyst decides on the type<br />
of classifier for a given mapping project, based on the informational requirements<br />
<strong>and</strong> resource availability along with the time constraints. Most remote sensing<br />
textbooks include detailed discussion on image classification algorithms. Products<br />
generated from these classification routines can be printed as maps or can be<br />
integrated in a GIS for further analyses. Since remotely sensed data are collected on<br />
a routine basis, periodic updates can be generated for any area <strong>and</strong> changes in l<strong>and</strong><br />
cover can be assessed.<br />
2.3. Geographic Information Systems (GIS)<br />
GIS is a computer-based system for storing, displaying, manipulating <strong>and</strong> analyzing<br />
geographic data, that can be tied to a geographic location to be described as<br />
geographic data. For example, the number of locust egg-pods (data) collected in<br />
each county or district (geographic location) is termed as geographic data. GIS can<br />
store, <strong>org</strong>anize <strong>and</strong> analyze diverse sets of geographic data, such as the number of<br />
locust egg-pods, hopper b<strong>and</strong> or swarm density <strong>and</strong> area, temperature, rainfall<br />
received, vegetation at those sites <strong>and</strong> so on. Users can query a GIS in order to<br />
combine information from physical <strong>and</strong> environmental variables for any application.
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As physical <strong>and</strong> environmental conditions change, one can update the<br />
information stored in a GIS <strong>and</strong> generate new results in a relatively short time. For<br />
example, an analyst can select sites for field visits based on distance to roads <strong>and</strong><br />
vegetation types. Information on roads <strong>and</strong> vegetation types are stored separately (as<br />
spatial data layers) in a GIS <strong>and</strong> can be combined to generate new or derived<br />
information. It is possible to combine other variables (e.g. soil type, elevation values<br />
etc.) to narrow down the sampling sites. A thorough discussion on GIS is beyond the<br />
scope of this chapter, but numerous textbooks are available. Similarly, GIS software<br />
has also grown in number <strong>and</strong> functionality <strong>and</strong> some of the commonly used ones<br />
are listed in Table 4.<br />
Table 4. Selected examples of geographic information system (GIS) software.<br />
Software Manufacturer Website<br />
ArcGIS ESRI www.esri.com<br />
AutoCAD Autodesk www.autodesk.com<br />
Cartalink Clark Labs www.clarklabs.<strong>org</strong><br />
GeoMedia Intergraph www.intergraph.com<br />
GRASS US Army Labs www.cecer.army.mil<br />
MapInfo MapInfo www.mapinfo.com<br />
MicroStation Bently Systems www.bently.com<br />
TNTmips MicroImages Inc. www.microimages.com<br />
Surfer Golden Software www.golden.com<br />
Sage GIS DLSR www.dlsr.com.au<br />
GIS technology can be used for analyzing spatial patterns in insect populations.<br />
Georeferenced data about insect densities, crop type, <strong>and</strong> soils for a location can be<br />
incorporated in a GIS for producing new map layers (Liebhold, Rossi, & Kemp,<br />
1993). A map layer, generally composed of only one type of data, thus has a theme.<br />
Furthermore, themes that represent similar areas can be combined to form a full GIS<br />
database. The GIS serves as a tool for analyzing interactions within <strong>and</strong> between the<br />
various spatially referenced data themes. Management <strong>and</strong> analysis of large spatial<br />
databases would be impossible without this type of software.<br />
GIS is being widely used in conjunction with remotely sensed data (satellite<br />
imagery) in Africa <strong>and</strong> Australia for mapping locust habitats (Bryceson, 1989;<br />
Cressman, 1997; Voss & Dreiser, 1997). FAO Scientific Advisory Committee<br />
considered GIS as the most appropriate technology to aid locust forecasters <strong>and</strong><br />
researchers (FAO, 1989). GIS is able to improve the specialists’ ability to assess <strong>and</strong><br />
interpret current <strong>and</strong> historical data on locusts <strong>and</strong> the environment (Healey,<br />
Robertson, Magor, Pender, & Cressman, 1996). Since Desert locust records are<br />
among the most complete which exist for an insect pest, a specific GIS “SWARMS”<br />
(Schistocerca WARning Management System) has been developed offering<br />
researchers <strong>and</strong> decision makers improved information for studying population<br />
dynamics <strong>and</strong> for displaying <strong>and</strong> testing alternative control strategies (Cressman,<br />
1997; Magor & Pender, 1997).
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GIS techniques have also been applied to grasshopper ecology in temperate<br />
regions, especially in the US. In Montana, with the use of GIS, regional spatiotemporal<br />
grasshopper outbreak characteristics have been examined (Kemp, Kalaris,<br />
& Quim<strong>by</strong>, 1989; Cigliano, Kemp, & Kalaris, 1995). In Wyoming, GIS was<br />
implemented to reveal the historic spatial characteristics of grasshopper outbreaks<br />
(1960–1993), as well as for spatial analysis of ecological factors related to<br />
grasshopper population dynamics (Schell, 1994; Lockwood & Schell, 1995). Schell<br />
(1994) studied the spatial properties of grasshopper infestations in Wyoming <strong>and</strong><br />
found that 72% of grasshopper outbreaks are confined to a particular soil type which<br />
has a very limited distribution range (1% of the state). Thus, the GIS analysis<br />
revealed that a certain ecological factor was highly correlated with the potential of a<br />
habitat to support an outbreak. The results of this study contributed greatly to the<br />
optimization of grasshopper survey <strong>and</strong> management in the state (Schell &<br />
Lockwood, 1995, 1997a, 1997b).<br />
2.4. Global Positioning Systems (GPS)<br />
GPS is used, among applications, for determining geographic coordinates while<br />
collecting data in the field. GPS consists of a constellation of satellites that transmit<br />
signals which are received <strong>by</strong> h<strong>and</strong>-held units called GPS Receivers, that can<br />
process the signals <strong>and</strong> determine precise geographic position. Time taken for these<br />
signals to travel from each satellite to the GPS receiver is used for computing the<br />
distance to each satellite. A minimum of 3 distance measures from 3 different<br />
satellites are required to determine a geographic position on the surface of the earth.<br />
Sophisticated GPS Receivers can simultaneously receive signals from 8 or more<br />
GPS satellites <strong>and</strong> therefore compute geographic coordinates with higher accuracy.<br />
Based on the precision <strong>and</strong> sophistication GPS Receivers are categorized as<br />
recreational, mapping <strong>and</strong> survey grade GPS. Survey grade GPS Receivers are<br />
expensive <strong>and</strong> provide very accurate measurements, in comparison to the other<br />
grades of receivers.<br />
GPS technology is widely used for navigation <strong>and</strong> surveys. Relatively<br />
inexpensive receivers are used in recreational activities while more precise GPS<br />
receivers are used for navigating emergency <strong>and</strong> transportation vehicles <strong>and</strong> to<br />
obtain their whereabouts in real time. GPS technology is used in field data collection<br />
for applications such as locating sampling sites or insecticide-treated areas.<br />
Previously researchers would mark these locations on a printed map to associate<br />
their samples to geographic space. With the help of GPS technology, researchers can<br />
record the geographic coordinates while collecting field data <strong>and</strong> later they can<br />
export the coordinates to image processing or GIS software. This process eliminates<br />
errors associated with transcribing field notes <strong>and</strong> annotated coordinates in maps.<br />
Several national <strong>and</strong> international agencies use GPS technology for collecting<br />
periodic information about events on a near-real time basis. Such methods, in<br />
addition to reducing the errors associated with transcribing, reduce the time required<br />
to generate updated information from field data obtained periodically.
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3. REMOTE SENSING AND LOCUST PEST MANAGEMENT<br />
Remotely sensed data collected from airplanes <strong>and</strong> satellites have been used<br />
for mapping locust habitats <strong>and</strong> also for assessing the damages to vegetation<br />
following a locust outbreak. Individual aerial photographs often cover smaller area<br />
on the ground in comparison to the area covered <strong>by</strong> moderate resolution satellite<br />
images such as L<strong>and</strong>sat (Table 2). The geographic area of some coarse resolution<br />
satellite images such as AVHRR <strong>and</strong> MODIS cover several thous<strong>and</strong> square km.<br />
Ability to monitor or map large geographic areas is particularly appealing for<br />
assessing locust damages in remote regions of the earth. Showler (2003) categorized<br />
the applications as strategic or tactical. Strategic applications include mapping<br />
potential or actual locust habitats <strong>and</strong> using that information to devise suitable<br />
prevention measures e.g., chemical treatments. Tactical applications include<br />
monitoring ongoing locust plagues from aerial platforms or assessing damages to the<br />
vegetation following locust outbreaks. Following sections focus on the habitat<br />
requirements <strong>and</strong> lessons learned from using remotely sensed data <strong>and</strong> technology<br />
for either mapping locust habitats (strategic) or assessing damages (tactical)<br />
following locust outbreaks.<br />
In the domain of locust pest management, remote sensing has been used for the<br />
detection of changes in vegetation <strong>and</strong> the measurement of certain meteorological<br />
parameters. For example, satellite images were used to detect zones of green<br />
vegetation (temporarily mesic habitats activated after sporadic rains) which had the<br />
potential for colonization <strong>by</strong> locust populations in xeric l<strong>and</strong>scapes of Africa<br />
(Cherlet, Di Gregorio, & Hielkema, 1990; Cherlet & Di Gregorio, 1993; Voss &<br />
Dreiser, 1994, 1997) <strong>and</strong> Australia (McCulloch & Hunter, 1983; Bryceson &<br />
Wright, 1986; Bryceson, 1989). With its broad infrared electromagnetic spectrum,<br />
the TM sensor of the L<strong>and</strong>sat satellite appears to be a useful instrument for detecting<br />
different vegetation communities <strong>by</strong> their reflection in the l<strong>and</strong>scape <strong>and</strong> mapping of<br />
locust habitats at scales up to 1:100,000 (Voss, Drieser, & Popov, 1992, 1993a,<br />
1993b, 1994).<br />
As for the detection of the entomogenic effects on the vegetation, satellite<br />
imagery has proved to be useful in forest entomology (Dottavio & Williams, 1983;<br />
Rencz & Nemeth, 1985). It also has potential for determining the crop losses due to<br />
locusts (Wewetzer, Krall, & Schultz, 1993). An attempt to use satellite imagery in<br />
the context of rangel<strong>and</strong> grasshopper ecology (Schell & Lockwood, 1996) strongly<br />
suggested that combinations of thermal <strong>and</strong> infrared wavelengths can distinguish<br />
infested l<strong>and</strong>s from the surrounding areas. Thus, active infestations are apparently<br />
revealed <strong>by</strong> a combination of entomogenic effects, including: (1) more rapid heating<br />
of the habitat, perhaps due to increased exposure of soils upon removal of forage <strong>by</strong><br />
grasshoppers (thermal), (2) decreased plant/soil moisture, perhaps as a consequence<br />
of grasshopper feeding (mid-infrared), <strong>and</strong> (3) changes in plant cell structure,<br />
perhaps as a consequence of herbivory-induced stress (near-infrared). A<br />
characteristic “halo” effect has been found with active outbreaks, which suggests a<br />
gradient of forage loss emanating from a high-density locust b<strong>and</strong>.<br />
Coupled with field observation, remote sensing can be employed to identify<br />
soils, vegetation <strong>and</strong> l<strong>and</strong> use characteristics, <strong>and</strong> from this initial information,
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173<br />
potential <strong>and</strong> active outbreak areas can be identified. The objective is to discriminate<br />
vegetation areas from bare soil <strong>and</strong> to monitor the changes in vegetation densities<br />
<strong>and</strong> qualities over time. This is achieved using specific indices, such as the<br />
Normalized Difference Vegetation Index (NDVI) (Tucker, Hielkema, & Roffey,<br />
1985). The methodology is well developed in Africa. An application of this method<br />
allowed identification of potential habitats of the Desert locust from remotely sensed<br />
data (Tappan, Moore, & Knausenberger, 1991; Cherlet & Di Gregorio, 1993) <strong>and</strong> to<br />
create corresponding habitat maps (Voss & Dreiser, 1997).<br />
3.1. Desert Locust Biology <strong>and</strong> Habitat Requirements<br />
The invasion area of the Desert locust (Schistocerca gregaria) occupies 29 million<br />
km 2 in Africa, S. Europe <strong>and</strong> SW Asia. During recessions, when population<br />
densities are low, the Desert locust inhabits arid <strong>and</strong> semi-arid l<strong>and</strong>s covering 16<br />
million km 2 from the Atlantic Ocean to NW India (COPR, 1982). Breeding occurs<br />
in the areas with 20–25 mm direct rainfall. Preferred oviposition sites are in s<strong>and</strong>y<br />
soils with a mosaic of grasses, herbs <strong>and</strong> shrubs. Although rain over the area is<br />
largely erratic, it tends to fall seasonally. Consequently locust breeding also takes<br />
place seasonally in different geographic locations (Fig. 1). The summer breeding<br />
zones include the Sahel, West Africa, Sudan, Eritrea, Ethiopia, <strong>and</strong> the India-<br />
Pakistan border. The winter/spring breeding zones include NW Africa, Iran,<br />
Pakistan, the Red Sea <strong>and</strong> the Gulf of Aden coasts, <strong>and</strong> the interior of Saudi Arabia<br />
<strong>and</strong> Yemen (FAO, 2001).<br />
Figure 1. Desert locust seasonal breeding zones <strong>and</strong> population movements<br />
between them (modified from FAO, 2001).<br />
Such complicated spatio-temporal pattern <strong>and</strong> an extremely large scale of the<br />
Desert locust population dynamics make its survey <strong>and</strong> forecasting extremely<br />
difficult. Furthermore, the pest’s breeding areas are often concentrated in very<br />
remote zones with low resident population or in the zones of the ongoing/imminent
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military conflicts such as Darfur, Ethiopia-Eritrea or India-Pakistan borders. Ground<br />
survey in such zones is difficult or impossible. The international cooperation<br />
between bordering countries is crucial, but it is not always in place for the efficient<br />
survey of the invasion area of the Desert locust which covers 65 countries.<br />
3.1.1. Habitat Mapping <strong>and</strong> Post-damage Assessment<br />
Pedgley (1974) was the first to apply satellite data to the Desert locust habitat<br />
monitoring. Tucker et al. (1985) recognized the potential of the remotely sensed data<br />
for the locust survey <strong>and</strong> forecasting. Hielkema (1981), Hielkema, Roffey, <strong>and</strong><br />
Tucker, (1986) <strong>and</strong> Ghaout (1990) used L<strong>and</strong>sat imagery to map vegetation in the<br />
critical locust’s gregarization areas in West Africa. Louveaux, Ghaout, <strong>and</strong> Gillon<br />
(1990) studied the functioning of the winter breeding area of the Desert locust in<br />
Mauritania using, among other techniques, the L<strong>and</strong>sat data. Successful<br />
implementation of a preventive Desert locust control strategy requires early <strong>and</strong><br />
reliable knowledge of areas where vegetation emerges after rainfall, providing<br />
suitable conditions for oviposition, egg hatching <strong>and</strong> hopper development. Cherlet<br />
<strong>and</strong> Di Gregorio (1993) tested the reliability of the NOAA AVHRR satellite data for<br />
these purposes. They attempted to calibrate different NOAA vegetation indices<br />
including NDVI, using extensive ground-collected field data from Niger. Their<br />
proposed calibration included two steps: (1) masking out the areas with no<br />
ecological potential for locust breeding; (2) correction of the vegetation index with a<br />
factor derived from the soil brightness. This methodology allowed the authors to<br />
detect some changes in the low cover vegetation. However, the lack of the<br />
background historical database on both, the vegetation <strong>and</strong> the locusts in certain key<br />
Desert locust breeding areas remains a major obstacle precluding the introduction of<br />
the remote sensing tools into the survey practice.<br />
Mapping of the Desert locust habitats using satellite imagery was done <strong>by</strong> the<br />
group of the late Prof. Dr. F. Voss in the 1990s. Dreiser (1994) used the L<strong>and</strong>sat<br />
Thematic Mapper data to produce the locust habitat maps for certain areas of Sudan,<br />
Mali <strong>and</strong> Mauritania at the scale of 1:200,000. Voss <strong>and</strong> Dreiser (1994) used the<br />
NDVI to detect the vegetated areas <strong>and</strong> then classified them with the maximum<br />
likelihood technique. The reliability of the resulting maps depended largely on the<br />
extensive ground observations <strong>and</strong> experience of the renowned locust expert Popov<br />
(1997) who participated in these studies. Such expertise is often unavailable in other<br />
Desert locust breeding areas which hinders the verification of the maps derived from<br />
satellite images. The authors concluded that the L<strong>and</strong>sat data were useful to assess<br />
the potential suitability of the Desert locust habitats. However, the actual habitats<br />
could be identified using higher temporal resolution imagery like NOAA AVHRR in<br />
combination with actual meteorological data from Meteosat <strong>and</strong> other similar<br />
satellites, which involve higher acquisition <strong>and</strong> processing costs (Voss & Dreiser,<br />
1997). Despl<strong>and</strong>, Rosenberg <strong>and</strong> Simpson (2004) used the vegetation indices<br />
derived from NOAA AVHRR data to connect the Desert locust gregarization <strong>and</strong><br />
b<strong>and</strong> formation areas in Mauritania <strong>and</strong> Sudan to l<strong>and</strong>scape structure. The authors<br />
concluded that the spatial resolution was insufficient to detect the initial
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175<br />
gregarization zones. Similarly, Babah Ebbe (2008) was not able to distinguish the<br />
vegetation from bare soil in Mauritania using the NDVI derived from the L<strong>and</strong>sat<br />
TM data. The author concluded that the very low vegetation density in the Saharan<br />
<strong>and</strong> Sub-Saharan zones does not allow for a reliable Desert locust habitat inventory<br />
using the L<strong>and</strong>sat tools. These findings are in line with those of the Desert Locust<br />
Information Service (DLIS) of the FAO UN which uses satellite data for forecasting<br />
locust outbreaks (http://www.fao.<strong>org</strong>/ag/locusts/en/activ/DLIS/satel/index.html).<br />
Until recently, DLIS relied on 1 km resolution SPOT-VGT imagery to monitor<br />
ecological conditions in a locust breeding areas. Although the sensor was<br />
specifically designed for vegetation monitoring, it has become clear that it is<br />
difficult to detect the sparse vegetation in the desert – vegetation that appears to be<br />
dry to the satellite yet, sufficiently green for Desert locust survival <strong>and</strong> breeding,<br />
resulting in under-prediction of the pest threat. Consequently, DLIS turned to higher<br />
resolution imagery, that of 250 m resolution MODIS, consisting of 16-day<br />
cumulative images. Analysis of individual channels provides an even more accurate<br />
estimation of ecological conditions in Desert locust habitats which are subsequently<br />
verified with survey results.<br />
Besides the vegetation, rainfall is another essential parameter necessary for<br />
accurate Desert locust forecast <strong>and</strong> risk assessment. DLIS uses rainfall estimates<br />
derived from METEOSAT, mainly infrared <strong>and</strong> visible channels, to underst<strong>and</strong><br />
better the spatial <strong>and</strong> quantitative distribution of rainfall in the Desert locust<br />
breeding areas. Although images are available every 15 min <strong>and</strong> estimates every<br />
three hrs, DLIS uses daily 24-h cumulative estimates as well as decadal estimates of<br />
rainfall processed <strong>by</strong> Columbia University's International Research Institute for<br />
Climate <strong>and</strong> Society (IRI). DLIS combines satellite-derived estimates with those that<br />
originate from meteorological models. Whenever possible, these are verified with<br />
ground data.<br />
DLIS collaborates with a variety of universities <strong>and</strong> other partner institutes such<br />
as the IRI, the Italian Institute of Biometeorology (IBIMET), the European<br />
Commission Joint Research Centre (JRC), NASA's World Wind Project, <strong>and</strong> the<br />
Catholic University of Louvain (Belgium) in improving the application of remote<br />
sensing imagery for Desert locust monitoring <strong>and</strong> forecasting. SPOT-VGT <strong>and</strong><br />
MODIS imagery is made available every 10 <strong>and</strong> 16 days respectively to locustaffected<br />
countries. These products are used to help guide national survey teams to<br />
potential areas of green vegetation where Desert locust may be present.<br />
Active remote sensing in the form of Vertically Looking RADAR (VLR) was<br />
used to observe the Desert locust flights over the Sahara as early as in 1968 (Roffey,<br />
1969). This technique provided novel measurements of aerial density, orientation,<br />
direction <strong>and</strong> speed of flight of solitarious locusts (Schaefer, 1969, 1976). Despite its<br />
very promising first results, the use of the RADAR devices for monitoring of the<br />
locust swarm migrations was considered impractical, mostly because of the timeconsuming<br />
nature of the data analysis (Reynolds, 1988; Riley, 1989). Subsequent<br />
attempts to use VLR showed its potential to distinguish between the flying Desert<br />
locusts <strong>and</strong> other insects (Smith, Riley, & Gregory, 1993). The obtained data could<br />
be a useful complement for the routine locust surveys (Riley & Reynolds, 1997;<br />
Chapman, Reynolds, & Smith, 2003).
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Finally, it is necessary to point out that currently available satellites are not able<br />
to directly detect individual locusts or locust swarms <strong>and</strong> hopper b<strong>and</strong>s. An attempt<br />
of Kibasa (2006) to detect the actual locust groups with the high-resolution Spot 5<br />
data failed, confirming that it was not possible to distinguish the insects from the<br />
background soil.<br />
With regard to the GIS applications, the analyses of the enormous amount of<br />
geospatial information collected <strong>by</strong> both, the satellites <strong>and</strong> field surveys from the<br />
vast geographic area of the Desert locust would be impossible without appropriate<br />
GIS tools (Hielkema & Snijders, 1994). The GIS SWARMS which was developed<br />
<strong>by</strong> the FAO in collaboration with Natural Resources Institute <strong>and</strong> the University of<br />
Edinburgh (UK) specifically for these purposes contains a number of databases<br />
including historical locust data for nearly 100 years, weather data, <strong>and</strong> background<br />
information such as soils <strong>and</strong> topography (Healey et al., 1996). SWARMS has been<br />
used operationally for locust early warning since 1996; it is being constantly revised<br />
<strong>and</strong> updated.<br />
One of the major hurdles in effective Desert locust forecasting is the collection<br />
<strong>and</strong> recording of data in the field <strong>and</strong> their subsequent transmission to a national<br />
locust center in near-real time. FAO DLIS developed, in collaboration with<br />
Novacom (France), a h<strong>and</strong>held device named eLocust2 for field locust officers<br />
(http://www.fao.<strong>org</strong>/ag/locusts/en/activ/DLIS/earlywarning/index.html) to enter <strong>and</strong><br />
send geo-referenced data in real time. The field officer enters <strong>and</strong> saves the data into<br />
a rugged h<strong>and</strong>held device which automatically determines the coordinates of the<br />
location of the survey or control operation using GPS technology. With a press of a<br />
button, the officer sends these data via satellite to the national locust center where<br />
they are received as an email attachment, downloaded, decoded <strong>and</strong> imported into a<br />
GIS. This GIS named RAMSES is used for the management <strong>and</strong> analysis of field<br />
results <strong>and</strong> of locust <strong>and</strong> environment data at a national level. eLocust2 data from<br />
the field are automatically imported into RAMSES <strong>and</strong> then are exported to FAO<br />
DLIS for further analysis, forecasting <strong>and</strong> early warning.<br />
Furthermore, FAO DLIS utilizes several specialized tools to supplement its<br />
analysis <strong>and</strong> forecasts (Ceccato, Cressman, Giannini, & Trzaska, 2007). A<br />
Trajectory Model (developed <strong>by</strong> Meteo Consult) estimates the source <strong>and</strong><br />
destination of swarm migrations forward <strong>and</strong> backward in time. Rainfall estimates<br />
<strong>and</strong> MODIS satellite imagery provided <strong>by</strong> IRI at Columbia University (New York,<br />
USA) are used to try to underst<strong>and</strong> where it has rain <strong>and</strong> where vegetation is green<br />
in the desert. Seasonal predictions of temperature <strong>and</strong> rainfall 6 months in advance<br />
are analyzed. Another model is used that estimates the developmental times of<br />
locust eggs <strong>and</strong> hoppers. The use of these tools in combination with the GIS allows<br />
the best possible analysis from which forecasts <strong>and</strong> early warning can be issued.<br />
Another tool potentially useful for locust forecasting is geostatistics.<br />
Woldewahid (2003) used geostatistics to predict the Desert locust densities at distant<br />
locations in the Red Sea coastal plains of Sudan, <strong>by</strong> spatial interpolation through<br />
kriging. He found a strong relationship between the Desert locust densities <strong>and</strong> the<br />
millet cropl<strong>and</strong>s despite the fact that these cropl<strong>and</strong>s occupied only a limited<br />
proportion of the study area (5%).
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3.2. Migratory Locust Biology <strong>and</strong> Habitat Requirements<br />
Migratory locust Locusta migratoria has the largest distribution area among all<br />
grasshoppers <strong>and</strong> locusts covering almost entirely the temperate <strong>and</strong> tropical zones<br />
of the eastern hemisphere (Fig. 2). Yet the ecological requirements of the species are<br />
rather narrow. Within this vast range the locust breeding areas are restricted to<br />
grassl<strong>and</strong>s on light soils, often in the wetl<strong>and</strong>s with reed st<strong>and</strong>s along rivers or lakes.<br />
There are about 10 subspecies or geographic races of the Migratory locust slightly<br />
differing biologically <strong>and</strong> morphologically (COPR, 1982). The tropical races<br />
develop continuously without diapause, while the temperate ones are univoltine.<br />
3.2.1. Habitat Mapping <strong>and</strong> Post-damage Assessment<br />
To date, remote sensing tools were applied to habitat mapping <strong>and</strong> damage<br />
assessment for two subspecies, L. m. migratoria in Central Asia <strong>and</strong> L. m.<br />
manilensis in China. In Kazakhstan <strong>and</strong> Uzbekistan, remotely sensed data collected<br />
from satellite platforms were used for mapping potential habitats of the Asian<br />
Migratory locust L. m. migratoria (AML). Throughout Central Asia, the AML<br />
spends most of its life cycle in common reed (Phragmites australis) st<strong>and</strong>s, usually,<br />
in river deltas.<br />
Figure 2. Distribution area of the subspecies of the Migratory locust Locusta<br />
migratoria (modified from COPR, 1982 <strong>by</strong> Latchininsky et al., 2002). Locusta<br />
migratoria migratoria <strong>and</strong> other northern subspecies___; L. m. cinerescens - - - ; L. m.<br />
burmana •••••; Indian subspecies …-; L. m. migratorioides - . - . L. m. capito …+…;<br />
Arabian subspecies ++++; L. m. manilensis ….; Australian subspecies -+-+-.<br />
To identify the AML habitats, one approach is to map the reed distribution<br />
annually or at specific times of the year coinciding with AML developmental stages<br />
(e.g., hatching of eggs or oviposition). Sivanpillai, Latchininsky, Driese, <strong>and</strong>
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Kambulin (2006), <strong>and</strong> Sivanpillai <strong>and</strong> Latchininsky (2007) demonstrated the utility<br />
of information derived from L<strong>and</strong>sat <strong>and</strong> MODIS satellites to estimate reed<br />
distribution in the River Ili (Kazakhstan) <strong>and</strong> Amudarya River (Uzbekistan) deltas<br />
respectively. Results from these studies showed that satellite data could accurately<br />
map the reed st<strong>and</strong>s when they are dominant (>80% classification accuracy).<br />
However, satellite data had relatively lower accuracy in detecting reeds growing<br />
together with other vegetation like shrubs <strong>and</strong> sedges (Latchininsky, Sivanpillai,<br />
Driese, & Wilps, 2007; Sivanpillai & Latchininsky 2008). Navratil (2007) used the<br />
higher resolution multispectral data collected <strong>by</strong> the SPOT satellite (Table 2) to map<br />
the reed distribution for a portion of the Amudarya River delta. L<strong>and</strong>sat Thematic<br />
Mapper 5 data could be used for mapping emerging reeds in the spring<br />
(Latchininsky et al., 2007). This time period coincides with the hatching of AML<br />
eggs <strong>and</strong> the satellite-derived information could be used for directing the ground<br />
survey towards potential nymphal habitats. Distribution of reeds coinciding with the<br />
locust oviposition (late summer) was mapped <strong>by</strong> Sivanpillai <strong>and</strong> Latchininsky<br />
(2008). Such information could be used for locating locust egg-beds. Satellitederived<br />
information could assist the government pest management agencies to<br />
devise treatment plans. Since satellites collect data on a regular basis, reed<br />
distribution maps can be updated periodically, providing basis for targeted locust<br />
surveys <strong>and</strong> treatments.<br />
Satellite data acquired prior <strong>and</strong> after an outbreak have been used for quantifying<br />
damages to vegetation. Ji, Xie, Li, Li, <strong>and</strong> Zhang (2004) used the pre- <strong>and</strong> postdamage<br />
MODIS images for assessing the damages caused <strong>by</strong> the Oriental Migratory<br />
locust L. m. manilensis in China’s Hebei Province. Using the NDVI values derived<br />
from these images, the researchers were able to identify the affected areas. The extent<br />
of vegetation damage was grouped into light, moderate, <strong>and</strong> heavy damage categories.<br />
Although MODIS images have relatively coarse spatial resolution (250 m), it was<br />
possible to identify 89% of the impacted areas. The authors concluded that satellitederived<br />
information could be more efficient than the traditional ground surveys.<br />
Zha, Gao, Ni, <strong>and</strong> Shen (2005) assessed the utility of MODIS data acquired over<br />
the growing season for monitoring Oriental Migratory locust outbreak in China.<br />
Tian, Ji, Xie, Li, <strong>and</strong> Li (2008) repeated the work conducted <strong>by</strong> Ji et al. (2004) using<br />
L<strong>and</strong>sat ETM+ data <strong>and</strong> reported higher classification accuracies compared to<br />
MODIS data. Ma et al. (2005) used L<strong>and</strong>sat ETM+ data to assess damage to<br />
vegetation caused <strong>by</strong> L. m. manilensis in China’s Dagang region. The ground-based<br />
locust monitoring stations established in the 1950s were unable to survey the<br />
exp<strong>and</strong>ed infested areas. Using the Leaf Area Index values derived from pre- <strong>and</strong><br />
post-damage images, the authors demonstrated the value of satellite data for routine<br />
monitoring of vegetation condition. Tian et al. (2008) repeated the pre- <strong>and</strong> postdamage<br />
assessment work conducted <strong>by</strong> Ji et al. (2004) but using L<strong>and</strong>sat ETM+<br />
data, <strong>and</strong> reported a very high accuracy of 98% for determining the geographic<br />
extent of the locust damage. However, the accuracy was slightly lower (92%) when<br />
they attempted to categorize the severity of the locust damage from L<strong>and</strong>sat images.<br />
Using soil moisture indices derived from MODIS data, Liu et al. (2008)<br />
demonstrated significant differences in soil moistures during severe (2001–2002)
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179<br />
<strong>and</strong> moderate (2003–2004) outbreak years in 3 regions prone to Oriental Migratory<br />
locust outbreak in China.<br />
Applications that used satellite data for mapping Migratory locust habitats,<br />
assessing risks of infestation <strong>and</strong> evaluating vegetation damage were comparatively<br />
fewer than the number of applications that focused on Desert locust (Section 3.1) or<br />
the Australian Plague locust (Section 3.3).<br />
3.3. Australian Plague Locust<br />
Australian Plague locust Chortoicetes terminifera occurs throughout Australia (Fig.<br />
3). Its ideal habitats consist of a mosaic of bare ground for basking <strong>and</strong> egg-laying,<br />
short grass cover for feeding <strong>and</strong> taller sparse tussocks for night shelter (COPR,<br />
1982). The locust can produce three annual generations under favorable weather<br />
conditions, primarily sufficient moisture. Hoppers form dense b<strong>and</strong>s which move<br />
several 100 m per day. Plagues originate from several recession areas in SW<br />
Queensl<strong>and</strong>, Central New South Wales, <strong>and</strong> NW Victoria where locusts are always<br />
present. Usually the onset of the plague is triggered <strong>by</strong> abnormally heavy rains from<br />
late November to January in the recession areas of the Australian dry interior.<br />
From these outbreak centers the huge swarms of adults migrate into agricultural<br />
zones covering distances of several 100 km. Rangel<strong>and</strong> forage is the preferred food<br />
for the Australian Plague locust. Migrating swarms, however, inflict severe damage<br />
to cereal crops, vineyards, orchards <strong>and</strong> vegetable gardens.<br />
3.3.1. Habitat Mapping <strong>and</strong> Post-damage Assessment<br />
Breeding zones of the Australian Plague locust situated in remote <strong>and</strong> semi-desert<br />
locations, the Australian entomologists were among the first to use remotely sensed<br />
data for locust habitat mapping. One of the earlier attempts to relate information<br />
derived from L<strong>and</strong>sat data with locust data was conducted <strong>by</strong> McCulloch <strong>and</strong> Hunter<br />
(1983). This study demonstrated that locust presence was confined to the following<br />
three map classes: stony downs, stony plains <strong>and</strong> high-level flood plains. Further<br />
development of the remote sensing tools was done <strong>by</strong> Bryceson (1984): he was able<br />
to detect even small area of vegetative growth after rains with L<strong>and</strong>sat data.<br />
Bryceson <strong>and</strong> Wright (1986) used several L<strong>and</strong>sat images modelled the origin <strong>and</strong><br />
spread of the 1984 Australian Plague locust outbreak. In this study they concluded<br />
that it was feasible to use satellite data to monitor changes in vegetation condition<br />
which could then be associated with locust breeding areas.<br />
In yet another study, Bryceson (1989) used L<strong>and</strong>sat MSS data to track the eggbed<br />
areas of the Australian Plague locust in New South Wales. Furthermore, the<br />
author showed that satellite data were instrumental in identifying the source areas<br />
from which the locust plagues developed (Bryceson, 1990, 1991).
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Figure 3. Australian Plague locust habitat (shown as shaded areas) map (Courtesy: Dr.<br />
Hunter <strong>and</strong> Mr. Deveson, Australian Plague Locust Commission, Canberra, Australia).<br />
In Australia, locust monitoring <strong>and</strong> control are executed <strong>by</strong> a federal agency, the<br />
Australian Plague Locust Commission (APLC), specifically created for these<br />
purposes. This facilitated the introduction of the meteorological remotely sensed<br />
data into the practice of locust forecasting (Bryceson & Cannon, 1990; Bryceson,<br />
1993; Bryceson, Hunter, & Hamilton, 1993; Hamilton & Bryceson, 1993). Multiple<br />
information sources, including remotely sensed vegetation <strong>and</strong> weather data as well<br />
as locust infestation data, were integrated into a decision support system developed<br />
at APLC (McCulloch, Bie, & Spurgin, 1994; Deveson & Hunter, 2000, 2002;<br />
Deveson, 2001).<br />
Locust swarm migrations were tracked in Australia <strong>by</strong> active remote sensing in<br />
the form of vertically-looking RADAR (Drake, Harman, & Hunter, 1998; Drake<br />
et al., 2001; Deveson, Drake, Hunter, Walker, & Wang, 2005). The methodology
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181<br />
proved useful. However, high costs of the installation <strong>and</strong> maintenance of the<br />
RADAR stations precluded it from practical use.<br />
Hunter, McCulloch, <strong>and</strong> Spurgin (2008) demonstrated the possibility of detecting<br />
the locust nymphal b<strong>and</strong>s from a low-flying aircraft, as a useful survey option.<br />
Australia remains an international leader in the operational use of remote sensing<br />
<strong>and</strong> GIS applications in locust management.<br />
3.4. Other Locusts<br />
About a dozen other locust species exist in addition to those described in earlier<br />
sections <strong>and</strong> their distribution ranges often cover vast, sparsely populated <strong>and</strong><br />
remote areas. These locust species can cause economic <strong>and</strong> environmental impact<br />
similar to any of the locusts discussed above. For example, the Moroccan locust<br />
(Dociostaurus maroccanus) habitats extend over 10,000 km across N. Africa,<br />
Middle East <strong>and</strong> Central Asia. Moroccan locusts can destroy valuable agricultural<br />
crops <strong>and</strong> adversely impact the livelihood of farmers in these regions. Chemical<br />
treatments can be effective only if they are coordinated <strong>by</strong> all impacted countries.<br />
Similarly, the Central American locust (Schistocerca piceifrons piceifrons) poses a<br />
threat to agricultural operations in Mexico <strong>and</strong> neighboring countries. Other locusts<br />
affect South Africa, South America <strong>and</strong> Southeast Asia. National Plant Protection<br />
Agencies in these regions spend considerable amount of resources for monitoring<br />
<strong>and</strong> managing the locust populations every year.<br />
Applications of the remote sensing <strong>and</strong> GIS technologies for monitoring <strong>and</strong><br />
management of the locust species other than the Desert, the Migratory <strong>and</strong> the<br />
Australian plague locusts are very scarce. To our knowledge, such studies were done<br />
for only two other locusts. Franc (2007) used high resolution SPOT satellite data to<br />
trace habitats of the Red locust Nomadacris septemfasciata in Madagascar.<br />
Comparing two SPOT images, one dated 1986 <strong>and</strong> the other dated 2004, he<br />
calculated the areas of deforested zones which served as migration pathways for this<br />
locust in the basin of the River Sofia. The accuracy of the image classification (77%;<br />
Kappa = 0.75) was verified through ground surveys. In 1986, the combined area of<br />
such “corridors” was 41,677 ha but as a result of intensive deforestation it increased<br />
to 67,607 ha <strong>by</strong> 2004. The newly cleared areas provided new migration pathways for<br />
the Red locust which produced spectacular outbreaks in the early 2000s for the first<br />
time ever in Madagascar.<br />
Sivanpillai, Latchininsky, Peveling, <strong>and</strong> Pankov (2009) used the Indian Remote<br />
Sensing (IRS) P6 Satellite –Advanced Wide Field Sensor (AWiFS) data to map the<br />
Italian locust Calliptamus italicus habitats in a very heterogenic l<strong>and</strong>scape of NE<br />
Kazakhstan, consisting of active <strong>and</strong> fallow cropl<strong>and</strong>s, shrub l<strong>and</strong>s, grassl<strong>and</strong>s <strong>and</strong><br />
riparian zones. This locust species inhabits primarily ab<strong>and</strong>oned agricultural fields<br />
(fallows) covered with sagebrush (Artemisia spp.) <strong>and</strong> other broadleaved weeds.<br />
Despite its relatively coarse spatial (56 m) <strong>and</strong> spectral (4 b<strong>and</strong>s) resolutions, the<br />
AWiFS data were sufficient to identify most l<strong>and</strong>scape features.
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CONCLUSIONS<br />
The idea of using remotely sensed data to identify locust habitats became plausible<br />
with the introduction of non-military satellites in the 1970s. Distribution ranges of<br />
many locust species cover vast, sparsely populated <strong>and</strong> remote areas, <strong>and</strong> the<br />
satellite data appeared to be tailor-made to address the spatio-temporal extent of the<br />
locust habitats. However, in the last two decades of the twentieth century, the<br />
practical use of the satellite data was impeded <strong>by</strong> inadequate computational<br />
hardware capacities <strong>and</strong> lack of specialized training for locust specialists in remote<br />
sensing data acquisition <strong>and</strong> processing. Hence, after a period of over-enthusiastic<br />
claims <strong>and</strong> views of the remote sensing as a panacea for solving locust problems, the<br />
research reports in the beginning of the 2000s sounded more cautious, if not<br />
skeptical (Despl<strong>and</strong> et al., 2004; Tratalos & Cheke, 2006). In the present chapter we<br />
attempted to summarize the most important achievements <strong>and</strong> drawbacks of the<br />
applications of the remote sensing <strong>and</strong> GIS technologies to locust monitoring <strong>and</strong><br />
risk assessment. Out of about a dozen locust species worldwide, this technology has<br />
been developed for only three species, the Desert, the Migratory, <strong>and</strong> the Australian<br />
Plague locusts. Numerous advances have been made in the use of satellite remote<br />
sensing data for monitoring the Desert locust habitats in Africa. Similarly, the<br />
habitats of the Australian Plague locust are being monitored through satellites, aerial<br />
photographs <strong>and</strong> RADAR imaging (active remote sensing) technologies. Satellite<br />
data from different platforms were used for habitat monitoring <strong>and</strong> crop loss<br />
assessment for the Migratory locust in Asia. For two other species, the Red <strong>and</strong> the<br />
Italian locusts, only pilot studies were done in this domain.<br />
The use of remotely-sensed information including the data from meteorological<br />
satellites became a routine part of the forecasting done <strong>by</strong> the FAO UN Desert locust<br />
Information Service (DLIS). Yet the efficacy of the forecasts is challenged <strong>by</strong> the<br />
vast geographic extent of the monitored territory of the Desert locust recession area<br />
(16 million km 2 ) <strong>and</strong>, consequently, <strong>by</strong> the huge amount of information to be<br />
collected <strong>and</strong> processed in near-real time (Van Huis, Cressman, & Magor, 2007).<br />
Habitats of the Migratory locusts, which are confined to reeds around water<br />
bodies, can be identified even with satellite platforms of relatively coarse spatial<br />
resolution (e.g. MODIS). Continuous reed st<strong>and</strong>s are easily distinguishable<br />
spectrally from other l<strong>and</strong> cover classes except when the reeds are mixed with<br />
shrubs of other vegetation. For such cases a higher temporal resolution of satellites<br />
with a shorter revisiting time is instrumental in following the phenological changes<br />
in the vegetation throughout the growing season.<br />
The Australian Plague locust management is implemented <strong>by</strong> the governmental<br />
entity, the APLC, which uses satellite <strong>and</strong> GIS technologies for locust monitoring<br />
<strong>and</strong> forecasting across a vast area of inner Australia. This country was one of the<br />
pioneers in practical introduction of the remote sensing as well as other technologies<br />
such as RADAR <strong>and</strong> aerial photography in locust population management.<br />
Applications of remote sensing <strong>and</strong> GIS technologies for mapping <strong>and</strong><br />
monitoring the habitats of most other locusts throughout the world lag behind. Some<br />
of these habitats are situated in active agricultural areas of countries such as<br />
Kazakhstan, Uzbekistan <strong>and</strong> Mexico. Locust pest outbreaks in these areas adversely
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183<br />
impact the economy <strong>and</strong> environment. Governments of these countries either<br />
independently or jointly (with their neighbors) are engaged in periodic monitoring<br />
<strong>and</strong> treatments to control locust populations <strong>and</strong> prevent them from damaging<br />
agricultural crops. Recently, efforts are underway to form a group of Central Asian<br />
<strong>and</strong> Caucasian countries to coordinate the locust population monitoring <strong>and</strong> control<br />
activities.<br />
Future locust habitat monitoring <strong>and</strong> surveying activities should incorporate<br />
remote sensing <strong>and</strong> GIS technologies for optimizing the resources available in these<br />
countries. Future work should also focus on testing the utility of remotely sensed<br />
data for mapping <strong>and</strong> monitoring the habitat of locust species that are yet to be<br />
studied. It is also encouraging that both the number of remote sensing satellites <strong>and</strong><br />
the countries that launch them have increased since early 1970s. In addition to<br />
government agencies several private companies have also launched remote sensing<br />
satellites that are collecting data for different parts of the world. With this increased<br />
availability of remotely sensed data (Table 2), users have a wide range of choice in<br />
terms of spatial, spectral <strong>and</strong> temporal resolutions while selecting imagery for a<br />
particular application. For example, images can be acquired more frequently <strong>by</strong><br />
obtaining data from different remote sensing satellites with complementary spatial<br />
<strong>and</strong> spectral resolutions (Section 2) providing the required information about locust<br />
habitat. Plant protection agencies <strong>and</strong> international <strong>org</strong>anizations must capitalize on<br />
these developments in terms of increased data availability.<br />
With more <strong>and</strong> more remotely sensed data distributed via the internet the time<br />
associated with obtaining the data has reduced tremendously. Previously data were<br />
mailed in tapes <strong>and</strong> discs <strong>and</strong> it could take several weeks thus reducing its<br />
usefulness. It is also important to note that not all countries or regions have access to<br />
high-speed internet. However, most remote sensing data can be downloaded directly<br />
from the satellites to ground receiving stations <strong>and</strong> processed in any country or<br />
region, thus avoiding the need to transfer large volumes of data through internet.<br />
Such activities require collaboration among international agencies (i.e., FAO),<br />
impacted countries, <strong>and</strong> satellite data vendors <strong>and</strong> agencies.<br />
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8<br />
PLANT DEFENSES AGAINST INSECT HERBIVORY<br />
FARHA-REHMAN 1 , FAREED A. KHAN 1 , SHOEBA B. ANIS 2<br />
AND S. M. A. BADRUDDIN 2<br />
1 Department of Botany, Aligarh Muslim University,<br />
Aligarh-202002, UP, India<br />
2 Department of Zoology, Aligarh Muslim University,<br />
Aligarh-202002, UP, India<br />
Abstract. Herbivory, the act of consumption of plant biomass <strong>by</strong> specialist animals, regulates the cycling<br />
of biotic <strong>and</strong> abiotic ecosystem components, through a complex process transferring materials among<br />
various trophic levels. Herbivores include insects <strong>and</strong> mammals of varying sizes, the former being most<br />
important due to their high diversity. Insects consume the biomass in varying proportions, depending on<br />
their size <strong>and</strong> density. Apparent checks <strong>and</strong> balances between prey <strong>and</strong> predators or hosts <strong>and</strong> parasites<br />
are chemically governed functions. Plants <strong>and</strong> herbivores receive <strong>and</strong> send signals to each other as well as<br />
to <strong>org</strong>anisms in higher trophic levels (predators) through volatile chemicals. Besides several<br />
morphological defence mechanisms, plants evolved specific chemical defences against insects. Among<br />
herbivores, insects also co-evolved mechanisms to overcome the volatile chemical arsenals of plants. In<br />
this review the role of plant defense against insect herbivory is discussed. The plant responses to repel<br />
insects <strong>and</strong> the synthesis of volatile chemicals to attract predatory insects or parasites are reviewed. Plants<br />
evolved genes (activated on insect attack) inducing the secretion of volatile chemicals. Such signalling<br />
attracts predators or parasites <strong>and</strong> is absent in plants when they are experimentally injured. Signalling is<br />
caused <strong>by</strong> the reaction with elicitors contained in the oral secretions of herbivorous insect. Through<br />
chemically operated keys, plants <strong>and</strong> insects regulate ecosystem functioning, allowing co-existence in<br />
wild <strong>and</strong> natural ecosystems.<br />
1. INTRODUCTION<br />
Agriculture is one of the major sectors of the Indian economy, since about 70% of<br />
human population is dependent on it for livelihood, other than food. The agriculture<br />
sector contributes over 40% of the gross national production, but food production<br />
has always remained a matter of great concern. During the past few months, the<br />
inadequate grain production has added to the global concern. Among other threats to<br />
crop productions, herbivorous insects <strong>and</strong> pests pose a very serious threat to plants<br />
in India, as well as all over the world.<br />
Herbivory, the feeding on living plants <strong>by</strong> animals or insects, is a key ecosystem<br />
process whose widely recognized effects on primary production, vegetation structure<br />
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A. <strong>Ciancio</strong>, K.G. Mukerji (eds.), Integrated Management of Arthropod Pests<br />
<strong>and</strong> Insect Borne Diseases, Integrated Management of Plant Pests <strong>and</strong> Diseases 5,<br />
DOI 10.1007/978-90-481-8606-8_8, © Springer Science+Business Media B.V. 2010
190<br />
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<strong>and</strong> composition depend on the type <strong>and</strong> intensity of feeding. Different types of<br />
herbivory affect several plant tissues, besides affecting primary production,<br />
translocation <strong>and</strong> accumulation of photosynthates to varying degrees. Herbivory<br />
affects a variety of ecosystem properties, primarily through differential changes in<br />
survival, productivity <strong>and</strong> growth of plant species.<br />
In evolutionary terms, the rise of insects represented a major selective force on<br />
plants evolution, <strong>and</strong> led to the selection of plants <strong>by</strong> their ability to generate<br />
defensive adaptations. Insect herbivores are mostly m<strong>and</strong>ibulated that either bite or<br />
chew vegetation. The rise of vascular plants led to the co-evolution of sap-sucking<br />
feeders, <strong>and</strong> several other forms of herbivores such as leaf mining, gall forming <strong>and</strong><br />
nectar feeding insects. The study of plant defense against insect herbivory is not<br />
only important from an evolutionary point of view, but is also useful in<br />
underst<strong>and</strong>ing the extent of its impact on agriculture, human <strong>and</strong> livestock food<br />
sources, as well as on the utility <strong>and</strong> survival of commodity plants or species of<br />
medicinal use. As an example of insects damage due to high rates of herbivory,<br />
grasshoppers feed on a wide range of plants <strong>and</strong> <strong>org</strong>anic material, <strong>and</strong> voraciously<br />
consume green forage approximately one-half of their body weight, every day.<br />
In the present review emphasis is given to herbivory <strong>and</strong> plant defense<br />
mechanisms, as well as to the chemical signalling among plants, herbivorous <strong>and</strong><br />
predatory insects. In fact, it is worth to determine these mechanisms before either<br />
using pesticides or employing other biotechnological means, i.e. genetically<br />
manipulated (GM) plants. It is known that the use of pesticides may indeed alter<br />
some ecosystem processes or introduce a structural change in density dependent or<br />
population regulation mechanisms, apart from the effects related to health hazard<br />
implications <strong>and</strong> costs. Finally, GM plants have several environmental <strong>and</strong><br />
ecological complications, including the developement of insect resistance in a way<br />
similar to resistance to some insecticides. Insect management is in effect a complex<br />
<strong>and</strong> difficult task, as suggested <strong>by</strong> the insects <strong>and</strong> plants co-evolution <strong>and</strong> survival<br />
for the past 97 million years (Lab<strong>and</strong>eira, Dilcher, Davis, & Wagner, 1994).<br />
2. PLANT DEFENSE MECHANISMS<br />
Plants curb insect herbivory <strong>by</strong> synthesizing <strong>and</strong> releasing complex blends of<br />
volatiles. Some of these compounds provide important host-location cues to predator<br />
insects or parasites, that are natural enemies of insect herbivores. Synthesis <strong>and</strong><br />
release of these chemical signals <strong>by</strong> attacked plants are active physiological<br />
processes, triggered <strong>by</strong> chemical elicitors or substances contained in the oral<br />
secretion of attacking herbivores. Certain chemicals contained in the saliva of<br />
grazing insect (herbivores) activate the synthesis <strong>and</strong> release of plant volatiles. The<br />
process of attracting predatory insects involves the interaction of specific blends of<br />
plant volatiles, with highly sensitive receptor molecules of the predators (De<br />
Moraes, Mescher, & Tumlinson, 2001).<br />
Plant volatiles represent a language through which attacked plants send signals<br />
to healthy plants in their vicinity <strong>and</strong> also invite predators or parasites of their<br />
herbivores. This adaptation is genetically fixed <strong>and</strong> controlled <strong>by</strong> a set of genes<br />
present in plants. In particular, a set of five defense genes are induced when a plant
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191<br />
is exposed to volatiles proceeding from nera<strong>by</strong> co-specific leaves infested with<br />
insects. All these genes were not induced in healthy plants when exposed to the<br />
blend of volatiles from artificially wounded leaves. At least three terpenoids in the<br />
infested leaves were responsible for the gene activation process, leading to the<br />
release of special blends of volatiles (Arimura et al., 2000).<br />
Volicitin, N-(17-hydroxylinolenoyl)-L-glutamine <strong>and</strong> β-glucosidase are elicitors<br />
of plant volatiles <strong>and</strong> are released only on insect chewing. Volacitin is a component<br />
of the oral secretion of beet worm caterpillars, which induce corn seedlings to<br />
synthesize <strong>and</strong> release volatile chemical signals. β-glucosidase is present in the<br />
regurgitant of Pieris brassicae caterpillar (Mattiacci, Dicke, & Posthumus, 1995).<br />
Generally, plant defenses can be categorized into two groups, such as constitutive<br />
<strong>and</strong> induced defenses. Constitutive defenses are always present in plants, while<br />
induced defenses are synthesized at or mobilized to the site of attack, when a plant is<br />
injured. Constitutive defenses range from mechanical defenses to the accumulation of<br />
digestibility reducers <strong>and</strong> toxins. Induced defenses include secondary metabolic<br />
products <strong>and</strong> may induce morphological <strong>and</strong>/or physiological changes. Both these<br />
defenses (inducible <strong>and</strong> constitutive) are known to increase the defensive ability <strong>and</strong><br />
effectiveness of attacked plants, against a wide range of insect herbivores.<br />
Wounding <strong>by</strong> herbivores activates the systemic expression of defense genes<br />
through the octadecanoid signal pathway. The insect saliva, containing chemical<br />
elicitors such as volicitin, also triggers the attacked plant to release a bouquet of<br />
volatile compounds which attract parasitic or predatory insects to check the<br />
attacking herbivore. Volicitin stimulates release of volatiles through the<br />
octadecanoid pathway <strong>and</strong> there<strong>by</strong> raises the possibility of cross talk between this<br />
molecule <strong>and</strong> the wound-induced expression of defense genes (Farmer, 1997).<br />
In controlled trials, corn seedlings <strong>and</strong> cotton plants damaged <strong>by</strong> caterpillars<br />
were observed to release volatiles attracting parasitic wasps, laying their eggs in the<br />
caterpillar’s body (Turlings, Tumlinson, & Lewis, 1990). The hatching eggs<br />
produced wasp larvae feeding on the host, which eventually killed the caterpillar.<br />
Over 15 plant species, 10 herbivore <strong>and</strong> 10 predatory insect species were observed<br />
to form a stable, tri-trophic food web (Takabayashi & Dicke, 1996).<br />
Another example of chemical signalling is given <strong>by</strong> nocturnal moths which lay<br />
their eggs on healthy plants, on which newly hatched larvae feed during day light.<br />
The plants attacked <strong>by</strong> the larvae were found to attract parasitic insects. In particular,<br />
De Moraes et al. (2001) reported that tobacco (Nicotiana tabacum) plants under<br />
attack from caterpillars produced two different blends of volatiles during night or<br />
day periods. The night time blends of volatiles were small, unsaturated derivatives<br />
of fatty acids <strong>and</strong> discouraged pregnant nocturnal herbivore moths (Heliothis<br />
virscens) for laying eggs. Night time herbivory food chain was thus discouraged, to<br />
avoid further plant damage (De Moraes et al., 2001). At the same time, repelling the<br />
night time pregnant moths <strong>by</strong> a specific blend of volatiles also reduced caterpillars<br />
competition with other day time herbivorous insects <strong>and</strong> also the attacks on their<br />
larvae <strong>by</strong> the predators already invited <strong>by</strong> diurnal caterpillars. It is important to note<br />
that the hatching larvae of nocturnal moths feed during the day time. However, it is<br />
not clear whether the night time blends of volatiles are specifically produced or if
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FARHA-REHMAN ET AL.<br />
they are <strong>by</strong>-products of diurnal volatiles (De Moraes et al., 2001). The dual function<br />
of volatiles released on herbivores attack is believed to have evolved<br />
simultaneously. The release of night time blends of volatiles of tobacco plant are<br />
also constituents of the set of volatiles released during attacks from diurnal insects,<br />
<strong>and</strong> defended tobacco plants from both diurnal <strong>and</strong> nocturnal herbivore caterpillars<br />
(De Moraes et al., 2001).<br />
If the full range of volatile signals used <strong>by</strong> plant to communicate with each<br />
other <strong>and</strong> with insects could be exploited, <strong>and</strong> its relevance in ecology also<br />
understood (including the identification of genes responsible for volatiles synthesis),<br />
plants could then be activated to emit specific blends of defensive volatiles at an<br />
appropriate day <strong>and</strong> night time, well before insects attack. The synthesis of these<br />
volatiles even in traces would then contribute to minimize the use of environment<br />
detrimental pesticides (Ryan, 2001).<br />
3. INSECT DIVERSITY AND CROP DAMAGE<br />
In spite of the fact that a large number of insect species are yet to be described <strong>and</strong><br />
reported, about 1.7 ⋅ 10 6 species of insects are already known, representing 56% of<br />
all members in the whole animal kingdom. According to another estimate, insects<br />
account for 64% of the whole animal biodiversity. Insects are known to have<br />
evolved several adaptation mechanisms making them one of the best fitting group in<br />
almost all climate <strong>and</strong> environment conditions (Atwal & Dhaliwal, 2003). The small<br />
body size, strong exoskeleton, high mobility through flight, efficient water<br />
conservation mechanism, rapid reproduction <strong>and</strong> resistance allowed their adaptation<br />
to diverse climates, <strong>and</strong> the maintenance of their own biodiversity. Honey bees, silk<br />
worm, Lac insect (pigment producers) <strong>and</strong> pollinators are also economically<br />
important species, as also the predators <strong>and</strong> parasites of herbivorous species. Their<br />
life cycle may be small, covering one season only, or last longer, for more seasons.<br />
There are varying reports concerning crop losses due to insect pests attacks. The<br />
losses caused <strong>by</strong> pests, diseases <strong>and</strong> weeds on a global scale are considered to vary<br />
between 35 <strong>and</strong> 37% (Atwal & Dhaliwal, 2003; Haq, Atif, & Khan, 2004; Brewer,<br />
2001). Crop losses due to various pest categories are very high in both developed<br />
<strong>and</strong> developing countries. In North America, Europe <strong>and</strong> Japan, estimates of crop<br />
losses are 10–30% (Atwal & Dhaliwal, 2003). However, crop losses due to pests are<br />
very high in developing regions. In India, estimated crop losses due to insect<br />
herbivores until a few decades ago were 18% for cotton, 10% for rice, 5% for<br />
oilseed <strong>and</strong> 5% for pulse crops (Atwal & Dhaliwal, 2003). Older (>50 years)<br />
estimates of crop losses due to insects ranged around 13%, whereas other pathogen<br />
losses averaged 12%. Arthropod pests, with more than 9,000 species including<br />
insects <strong>and</strong> mites, contributed towards major losses to agriculture crops, not only <strong>by</strong><br />
direct damages, but also acting as vectors <strong>and</strong> transmitting various plant diseases<br />
(Griswold, 1953). Among all grazers, insect herbivores account today for a 50% of<br />
total biomass consumption. Among all herbivores, insects are far most significant<br />
grazers as they co-evolved feeding strategies besides the deploy of plants<br />
defence mechanisms (Ehrlich & Ehrlich, 1970).
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193<br />
According to a recent report, insects may consume about 10–20% of a crop<br />
(Ferry, Edwards, Gatehouse, & Gatehouse, 2004). From previous global estimates,<br />
insect pests resulted in crop losses around $7 billion, while $3 billion annually were<br />
spent in the US on pest control efforts in the early sixties (Janick, Schery, Woods, &<br />
Ruttan, 1974). In India, Rangaswami (1983) estimated annual economic crop losses<br />
around Rs. 150 thous<strong>and</strong> million (≈ US$ 3191 million). Another estimate of total<br />
losses of field crops <strong>and</strong> food grain (pre <strong>and</strong> post harvest) caused <strong>by</strong> insects was<br />
around Rs. 336.6 billion (approx. US$ 7.17 billion) per year on a global scale (Atwal<br />
& Dhaliwal, 2003). Control of insect pests has hence a high potential in increasing<br />
crops production <strong>and</strong> farmers’ revenues, with a potential estimated increase of yields<br />
<strong>by</strong> 13.1–18.7 million tonnes per year. As an example, control of herbivory (flies <strong>and</strong><br />
pod borers) may reduce total crop damage up to 30%, with an increase of sugarcane<br />
yield <strong>by</strong> 20% or of groundnut production <strong>by</strong> 15% (Atwal & Dhaliwal, 2003).<br />
The loss to leaf area caused <strong>by</strong> herbivores varies from 4.8 to 32.5% (Lowman &<br />
Box, 1983). Chemical changes in leaf composition are also produced <strong>by</strong> insect<br />
attacks. For example, the insect attack may result into accumulation of phenolics<br />
which may reduce in turn grazing intensity <strong>by</strong> other species (Lowman & Box, 1983).<br />
In red alder (Alnus rubra), plant memories to insect attacks, in terms of the<br />
durability of chemical or physical defense, also varied depending on the feeding<br />
insect species (Williams & Myers, 1984).<br />
Further estimates of plant damage due to herbivory may be derived <strong>by</strong> assays on<br />
annual crops or observations on perennial plants. The loss of maize (Zea mays) to<br />
herbivory <strong>by</strong> the grasshopper Choroedocus illustris follows a density dependent<br />
pattern. The damage intensity to the leaf area due to adult grasshoppers varied from<br />
1.64 to 3.55% as 10, 20 <strong>and</strong> 40 adults attacked, respectively, 32.5, 60.9 <strong>and</strong> 79%<br />
leaves of all plants (Farha-Rehman, 2008). Furthermore, in damaged maize leaves,<br />
the insect attack during 15 days led to a proportionate loss of leaf proteins <strong>and</strong> an<br />
increase in proline accumulation (Farha-Rehman, 2008). In the insect herbivory on<br />
the Australian woodl<strong>and</strong> eucalypt (Eucalyptus blakelyi), Journet (1981) noted that<br />
herbivorous insects caused 40% annual foliage damage. The abscission of damaged<br />
foliage further enhanced the total annual foliage damage up to 70%.<br />
4.1. Insect Herbivores<br />
4. HERBIVORY<br />
Insects are the primary herbivores in many ecosystems <strong>and</strong> their size vary from the<br />
tiny aphids to very large species. They feed on a vast variety of plants, ranging from<br />
algae to angiosperms. The insect grazers form a complex system at the herbivory<br />
level in food webs. About 80% of plant material consumed <strong>by</strong> insects, <strong>and</strong> their<br />
secondary production, can equal or exceed the plant biomass consumed <strong>and</strong> rebuilt<br />
as secondary productivity <strong>by</strong> vertebrate grazers in grassl<strong>and</strong>.<br />
During the evolution of life on earth, insects have been the most significant<br />
herbivores <strong>and</strong> co-evolved with l<strong>and</strong> plants, since they are dependent on plants for<br />
food <strong>and</strong> shelter. The herbivores co-evolved mechanisms to obtain food from plants<br />
despite the set-up of a diverse range of plant defenses. Herbivore adaptations to
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plant defense have been attributed to the offensive traits linked with promoting<br />
increased feeding <strong>and</strong> use of a suitable host.<br />
Relationship between herbivores <strong>and</strong> their host plants often resulted in<br />
reciprocal evolutionary changes. For example, some herbivores co-evolved ways to<br />
hijack plant defenses <strong>by</strong> sequestering defensive chemicals <strong>and</strong> using the modified<br />
blend to protect themselves from predators.<br />
4.2. Plant Responses to Insect Herbivory<br />
A number of volatile chemicals produced <strong>by</strong> plants promote or reduce herbivory.<br />
The increase of nitrogen, stored as accumulated proline <strong>and</strong> valine residues, was<br />
observed to stimulate grasshopper herbivory during drought stress (Haglund, 1980).<br />
Experimental evidence suggested that grasshoppers detect <strong>and</strong> preferentially feed on<br />
grasses treated with the amino acid proline <strong>and</strong> valine, whose accumulation levels in<br />
plants commonly increase under drought. This adversity may lead to insect<br />
concentration on drought stressed plants (Haglund, 1980).<br />
Leaf toughness, total phenols <strong>and</strong> condensed tannins increased in the leaves of<br />
five tree species of Australian rain forest, because of insect grazing (Lowman &<br />
Box, 1983). In most of these trees leaf toughness <strong>and</strong> chemical toxicity increased<br />
with leaf aging, leading to a corresponding decrease in insect grazing. The herbivory<br />
caused leaf area losses between 4.8 <strong>and</strong> 32.5%, but losses were positively correlated<br />
with leaf toughness rather than phenolic contents. Lowman <strong>and</strong> Box (1983) inferred,<br />
from these findings, an interaction of factors including physical <strong>and</strong> chemical<br />
characteristics of leaves, with spatial <strong>and</strong> temporal factors that induced the variation<br />
in insect grazing intensities.<br />
Leaf structure <strong>and</strong> <strong>org</strong>anization may also protect plants from herbivores,<br />
although with complex outcomes. As an example, the tiny hooked trichomes on<br />
leaves <strong>and</strong> stems of Mentzelia punila (Family Loasaceae) entrapped <strong>and</strong> killed not<br />
only herbivore aphids (Macrosiphum mentzeliae) but also incapacitated a coccinellid<br />
beetle (Hippodamia convergens) that preys upon the aphid enemy (Eisner, Eisner, &<br />
Hoebeke, 1998).<br />
Besides leaf age, the pattern of herbivory may vary with the plant species.<br />
Intraspecific variation in the pattern of herbivory on young <strong>and</strong> mature leaves of<br />
Trichilia cipo (Meliaceae) <strong>and</strong> Cecropia insignis (Moraceae), two tropical trees, was<br />
observed in a lowl<strong>and</strong> rain forest in Panama. Mature leaves of Cecropia suffered a<br />
five fold greater damage than Trichilia, irrespective of the differences in life history,<br />
habitat, defensive characteristics <strong>and</strong> damage levels (Coley, 1983).<br />
4.3. Plant Reaction to Previous Herbivores<br />
The previous herbivore attack of Western tent caterpillar, Malacosoma californicum<br />
pluviale, on red alder was observed to improve food quality for fall webworm<br />
(Hyphantria cunea) larvae. Three hypothesis concerning the insect-plant interactions<br />
were tested <strong>by</strong> rearing fall webworm larvae in the laboratory on foliage collected<br />
from red alder trees, with different histories of western tent caterpillar herbivory.
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195<br />
Fall webworm larvae grew relatively faster, with heavier pupil weight, when raised<br />
on foliage with previous history of herbivory (caused <strong>by</strong> moderate densities of<br />
western tent caterpillar during two previous summers) in comparison to those fed on<br />
foliage from unattacked trees. This finding did not fit the hypothesis that previous<br />
history of herbivory induced the production of plant defensive chemicals in red<br />
alders. Growth patterns of webworms were the same, either fed on foliage from<br />
unattacked trees adjacent to those attacked <strong>by</strong> fall webworm larvae or on the foliage<br />
of red alder trees, growing at a longer distance from attacked trees. This study<br />
showed, however, that continued insect attacks can deteriorate the food quality of<br />
attacked trees (Williams & Myers, 1984).<br />
Seed consuming larvae reduced seed production in turtlehead, Chelone obliqua.<br />
Seed production was also reduced due to severe herbivory <strong>by</strong> specialist folivores<br />
(Stamp, 1987).<br />
Plant defense signalling can also be induced <strong>by</strong> biotic attacks. In some<br />
interactions, defense was enhanced prior to attack <strong>by</strong> another <strong>org</strong>anism, whereas in<br />
other species, signals were conflicting. Below ground attack may also influence<br />
responses to above ground attack <strong>and</strong> vice versa, due to systemic induction of<br />
defense metabolism pathways (Bruce & Pickett, 2007).<br />
4.4. Impact of Herbivory on Ecosystem<br />
In a study on the impact of insect herbivory on eight plant species (including<br />
perennial forbs <strong>and</strong> grasses), the size variability in plant populations influenced<br />
insect herbivory, which in turn affected the fitness of individuals under natural<br />
successions. The size variability was reduced with herbivores abundance. Insect<br />
herbivory reduced size <strong>and</strong> survival of plants as did competition, which directly<br />
affected the size <strong>and</strong> distribution of plants (Gange & Brown, 1989).<br />
Insect herbivory may also act as a plant population regulatory factor (Williams,<br />
1990). Herbivory limited the distribution of Eucalyptus pauciflora in sub-alpine<br />
forest in Australia which was replaced <strong>by</strong> E. dives due to increased herbivory<br />
preferences. The co-occurrence of E. dalrympheana with E. dives <strong>and</strong> E. pauciflora<br />
was maintained <strong>by</strong> a density-dependent stabilizing mechanism, caused <strong>by</strong> leaf<br />
parasites. The leaf damage <strong>by</strong> insect on the ligno-tuberous seedlings of these three<br />
subalpine eucalypts was not consistent, but the damage levels in the seedlings of E.<br />
dalrympleana were lower than those of E. pauciflora <strong>and</strong> E. dives (Williams, 1990).<br />
Insect herbivory <strong>by</strong> grasshoppers accelerated nutrient (nitrogen) cycling, plant<br />
production <strong>and</strong> abundance, <strong>and</strong> there<strong>by</strong> influenced plant species composition over a<br />
period of 5 years (Belovsky & Slade, 2000). Enhancement in plant abundance<br />
depended on consumption rate of grasshoppers <strong>and</strong>, under some conditions,<br />
grasshoppers decreased nutrient cycling <strong>and</strong> plant density (Belovsky & Slade, 2000).<br />
The nocturnal plant volatiles induced <strong>by</strong> caterpillars were observed to repel cospecific<br />
females (De Moraes et al., 2001). Tobacco plants released herebivore<br />
induced volatiles night <strong>and</strong> day. The volatile compounds released exclusively at<br />
night were highly repellent to female moths H. virescens. In fact, tobacco plant<br />
released temporarily different volatile blends <strong>and</strong> lipidopteran herbivores used night<br />
time plant volatile signals to select suitable oviposition sites. In night, attacked
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FARHA-REHMAN ET AL.<br />
tobacco plant released volatiles that repelled nocturnal pregnant moths looking for<br />
the site of oviposition. In the day, tobacco plants under attack <strong>by</strong> herbivores released<br />
blends attracting parasitic or predatory insects (De Moraes et al., 2001). These<br />
responses were beneficial for tobacco plants <strong>and</strong> the herbivorous insect involved<br />
(De Moraes et al., 2001). These findings indicate that host plant on one h<strong>and</strong><br />
attracted predators of herbivorous caterpillars during day time <strong>and</strong> female moth coevolved<br />
to avoid such plants for oviposition using some exclusive night time blends<br />
to avoid predators of larvae. This co-evolution between tobacco <strong>and</strong> pregnant female<br />
moth maintained ecosystem functioning.<br />
A co-evolutive adaptation was observed as the result of plant-insect interactions<br />
(Wittstock et al., 2004). For example, maize rapidly mobilizes the accumulation of a<br />
33-kDa cysteine protease in response to feeding of caterpillars, there<strong>by</strong> posing<br />
resistance to herbivory. The accumulation of the 33-kDa cystein protease in the maize<br />
midwhorl significantly reduced caterpillar growth due to impaired nutrient utilization<br />
(Pechan, Cohen, Williams, & Luthe, 2002). The larvae of the specialist insect, Pieris<br />
rapae (cabbage white butterfly, Lepidoptera) also appear adapted to the glucosinolatemyrosinase<br />
system, a defensive chemical arsenal of the host plants.<br />
Trotter, Cobb, <strong>and</strong> Whitham (2002) studied herbivory, plant resistance <strong>and</strong><br />
climate in the tree ring records <strong>and</strong> noted that interactions distorted climatic<br />
reconstructions. The resistance or susceptibility of pines to herbivore <strong>and</strong> climate<br />
interaction in the tree ring record were detectable, due to hereditary characteristics.<br />
These authors found that herbivory reduced tree rings growth <strong>by</strong> 25–35% <strong>and</strong><br />
distorted climate reconstruction on growth rings. Herbivory-induced changes also<br />
reduced preference <strong>and</strong> performance of a variety of insects for a diverse group of<br />
plants <strong>and</strong> ultimately increased their fitness in natural environments, as shown from<br />
studies on wild radish (Raphanus raphanistrum) (Agrawal, 1999).<br />
4.5. Herbivore Strategies<br />
Several factors affect herbivores feeding, including the type of available food <strong>and</strong><br />
the biochemical products released during feeding. For example, the lubber<br />
grasshopper (Romalea guttata) feeds on a wide range of plant species <strong>and</strong> produces<br />
a metathoracic defensive secretion containing primarily phenolics <strong>and</strong> quinones<br />
(Jones, Hess, Whitman, Silk, & Blum, 1987). When reared on onion (Allium<br />
canadense) <strong>and</strong> an artificial diet, it secreted volatiles with fewer compounds, in<br />
altered proportions as compared to a set of insects reared on diets from a diverse<br />
group of 26 plant species, including onion. The diet diversity appeared to have a<br />
major impact on the quality <strong>and</strong> quantity of the autogenous defensive secretions of<br />
this generalist herbivore, possibly due to changes in precursors availability, owing to<br />
a diverse diet <strong>and</strong>/or to diet restrictions, leading to a physiological stress caused <strong>by</strong><br />
partitioning of resources to defensive chemicals (Jones et al., 1987).<br />
Larvae of Spodoptera eridania preferred for its diet proteins of Lotus<br />
corniculatus, as compared to tannins (Briggs, 1990). The larvae were given a choice<br />
of L. corniculatus plants whose chemical profiles were altered <strong>by</strong> feeding on plants<br />
grown with nutrient fertilization, or with symbiotic nitrogen fixation as their only
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197<br />
nitrogen source. The larvae preferred protein rich leaves, rather than leaves with<br />
higher tannin contents (Briggs, 1990).<br />
The caterpillar regurgitants were found to amplify the production of the wound<br />
induced phytohormone jasmonic acid (JA), but not of nicotine in Nicotiana<br />
sylvestris (McCloud & Baldwin, 1997). It was noted that herbivory <strong>and</strong> mechanical<br />
damage increased the concentration of the wound-signal molecule (JA) <strong>and</strong> the<br />
defense metabolite (nicotine) in native tobacco plants. However, the larvae of<br />
M<strong>and</strong>uca sexta while feeding on damaged leaves modified the plant normal<br />
defensive metabolites <strong>by</strong> reducing systemic JA in roots <strong>and</strong>, subsequently, the<br />
nicotine content in the whole plant (McCloud & Baldwin, 1997).<br />
4.6. Simulation of Herbivory<br />
Several experimental assays attempted to simulate herbivory, in order to gain an<br />
insight on the potentials of the biochemical changes <strong>and</strong> signals induced. Realistic<br />
herbivory simulations in terms of plant responses were noted on combining 50% leaf<br />
area clipping <strong>and</strong> JA spraying on Solidago canadensis, rather than either clipping or<br />
JA spraying alone (Van Kleunen, Ramponi, & Schmid, 2004). Further experimental<br />
assays on tomato plants showed that JA is a useful plant elicitor for pest<br />
management (Thaler, 1999a).<br />
Pontoppidan, Hopkins, Rask, <strong>and</strong> Meijer (2005) compared the effect of artificial<br />
mechanical wounding with herbivory <strong>by</strong> diamond-back moth larvae on rapeseed,<br />
Brassica napus, showing that the changes observed in myrosinase binding protein<br />
<strong>and</strong> myrosinase transcript levels were reflected in protein levels. In a tri-trophic<br />
interaction including the bacterial phytopathogen Pseudomonas syringae, Cui et al.<br />
(2005) reported that the bacterium manipulated the systemic plant defense against<br />
pathogens <strong>and</strong> herbivores. It was noted that virulent strains of P. syringae induced<br />
systemic susceptibility to a secondary P. syringae infection in the host plant<br />
Arabidopsis thaliana (L.) Heynh. The P. syringae infection elicited systemic<br />
induced susceptibility caused <strong>by</strong> the production of coronatine (COR), a pathogenderived<br />
functional <strong>and</strong> structural mimic of JA, which in turn induced a systemic<br />
resistance to attacks <strong>by</strong> the insect Trichoplusia ni.<br />
Recent studies provided evidence for specificity in the elicitation of induced<br />
plant responses <strong>by</strong> different attackers, suggesting that the host suitability for<br />
colonizing herbivores may depend on the herbivore species that initially damaged a<br />
plant. For example, the existence of a plant-mediated competitive asymmetry<br />
between herbivore species on Solanum dulcamara showed the dynamic nature of<br />
plant resistance, <strong>and</strong> its potential role in <strong>org</strong>anizing <strong>and</strong> structuring herbivore<br />
communities (Viswanathan, Narwani, & Thaler, 2005).<br />
In simulating/testing of diet components, specific ingredients may be identified<br />
which play a significant role in herbivores selections. Konno et al. (2006) found that<br />
mulberry (Morus spp.) latex, rich in antidiabetic sugar-mimic alkaloids, affected<br />
caterpillars dieting. Some ingredients of the latex milky sap exudate present in veins<br />
of the mulberry leaves were highly toxic to caterpillars, other than the silkworm<br />
Bom<strong>by</strong>x mori, playing a key role in selectivity of insect herbivory. Finally, some<br />
ecological factors may also affect plant consumption <strong>by</strong> herbivores, as shown <strong>by</strong>
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FARHA-REHMAN ET AL.<br />
Simonetti, Grez, Celis, <strong>and</strong> Bustamante (2007) who studied the herbivory <strong>and</strong><br />
seedling performance in a fragmented temperate forest of Chile. These authors<br />
observed that forest fragmentation alters plant-animal interactions, including<br />
herbivory. The insects were found to be important herbivores in the Maulino forest<br />
<strong>and</strong> fragmentation had strong indirect effects on plant communities, as mediated<br />
through trophic interactions.<br />
5.1. Plant Defense Strategies<br />
5. DEFENSE STRATEGIES<br />
The proteinase inhibitors of tomato plants are known to provide a defense strategy<br />
against insect herbivory <strong>by</strong> the beet armyworm, Spodoptera exigua (Broadway,<br />
Duffey, Dearce, & Ryan, 1986). The insect herbivory rapidly reduced plant quality<br />
<strong>and</strong> in turn larval growth, as shown <strong>by</strong> the larval feeding on foliages from insect<br />
damaged <strong>and</strong> undamaged tomato plants. This feedback mechanism involved the<br />
induction of tomato proteinase inhibitors resulting from larval feeding, that<br />
systemically reduced leaf nutritive value (Broadway et al., 1986). In Verbascum<br />
thapsus, herbivory was directly related to age dependent leaf pubescence (Woodman<br />
& Fern<strong>and</strong>es, 1991), since less pubescent leaves, of older plants, were more<br />
frequently attacked than the more pubescent leaves, of younger plants. The leaf hairs<br />
acted both as a barrier against herbivores <strong>and</strong> also prevent water loss. Similar agespecific<br />
mechanical defenses are widespread <strong>and</strong> effective against generalized<br />
chewing insects, such as grasshoppers (Woodman & Fern<strong>and</strong>es, 1991).<br />
The effect of leaf feeding <strong>by</strong> the larvae of Samea multiplicalis, at densities of<br />
0.8 <strong>and</strong> 1.6 larvae per plant, severely damaged Salvinia molesta, a floating weed, <strong>by</strong><br />
reducing leaf area, plant weight <strong>and</strong> ramet numbers (Julien & Bourne, 1988). The<br />
root <strong>and</strong> rhizomes were spared <strong>by</strong> the moths allowing the plants to continue its<br />
growth, but the insect feeding altered the nitrogen balance in above <strong>and</strong> below<br />
ground plant parts (Julien & Bourne, 1988).<br />
Several experimental assays provided evidence for a key role played <strong>by</strong> JA <strong>and</strong><br />
jasmonate in plant defense mechanisms. McConn, Creelman, Bell, Mullet, <strong>and</strong> Browse<br />
(1997) noted that jasmonate is essential for insect defense in Arabidopsis. The<br />
signalling pathways mounting defenses against chewing insects were complex. Mutant<br />
plants containing negligible levels of jasmonate showed high mortality (≈ 80%) when<br />
attacked <strong>by</strong> larvae of Bradysia impatiens, whereas neighbouring wild type plants were<br />
largely unaffected. These experiments precisely defined the role of jasmonate as<br />
essential for the induction of biologically effective defense in plant-insect interactions.<br />
The herbivory on rape seed plants <strong>by</strong> cabbage stem flea beetles (Psylliodes<br />
chrysocephala) induced systemic changes in glucosinolate profile (Bartlet, Kiddle,<br />
Williams, & Wallsgrove, 1999). A similar change was noticed when JA was applied to<br />
the plants cotyledons, suggesting that JA synthesis was initially induced <strong>by</strong> herbivory<br />
which in turn induced a negative effect on subsequent herbivory (Bartlet et al., 1999).<br />
Thaler, Stout, Karban, <strong>and</strong> Duffey (2001) found that jasmonate-mediated plant<br />
resistance may affect a community of herbivores. Several proteins induced in tomato<br />
foliage following herbivore damage were linked to reductions in herbivore
HERBIVORY & PLANT DEFENSE<br />
199<br />
performance under laboratory condition (Thaler et al., 2001). This induced resistance<br />
often suppressed many communities of herbivores. The information on the plant<br />
biochemistry, insect preference, performance <strong>and</strong> abundance may hence be helpful in<br />
developing practical tools for insect management, through natural or induced plant<br />
defense mechanisms (Thaler et al., 2001).<br />
The amounts of signalling molecule may affect the efficacy of defense<br />
metabolites. Quantitative relationships between induced JA levels <strong>and</strong> volatile<br />
emissions in maize during Spodoptera exigua herbivory have been reported <strong>by</strong><br />
Schmelz, Alborn, Banchio, <strong>and</strong> Tumlinson (2003a). JA induced emission of indole<br />
<strong>and</strong> sesquiterpenes (volatiles) limited the plant ethylene emission <strong>and</strong> also controlled<br />
excessive volatile production. In another study (Schmelz, Alborn, & Tumlinson,<br />
2003b), volicitin from the herbivore oral secretion induced JA levels, <strong>and</strong><br />
sesquiterpene volatiles were more excessively stimulated in maize than through<br />
mechanical damage in absence of volicitin. Relatively more significant increase in<br />
ethylene levels were recorded during beet army worm herbivory, than either <strong>by</strong><br />
wounding or volicitin treatments (Schmelz et al., 2003b).<br />
Engelberth, Alborn, Schmelz, <strong>and</strong> Tumlinson (2004) reported that airborne<br />
signals alert plants against insect herbivore attack. Green leafy volatiles including<br />
six carbon aldehydes, alcohols <strong>and</strong> esters were commonly emitted <strong>by</strong> plants in<br />
response to mechanical damage or herbivory. These volatiles induced intact<br />
undamaged neighbouring corn seedlings to rapidly produce JA <strong>and</strong> emit<br />
sesquiterpenes. These green leaf volatiles played a key role in plant – plant<br />
signalling <strong>and</strong> plant-insect interactions. Heil (2004) reported that JA induced<br />
defenses in lima bean (Phaseolus lunatus) was beneficial under natural condition.<br />
Finally, Howe <strong>and</strong> J<strong>and</strong>er (2008) observed that herbivore insects use diverse<br />
feeding strategies to obtain nutrients from their host plants. Plants responded to<br />
herbivory with the production of toxins <strong>and</strong> defensive proteins that target<br />
physiological processes in the insect. This strategy appears as a highly dynamic form<br />
of immunity, initiated <strong>by</strong> the recognition of insect's oral secretions <strong>and</strong> emission of<br />
signals from injured plant cells.<br />
5.2. Plant Receptor Molecules<br />
Cowpea (Vigna radiata) attacked <strong>by</strong> the fall armyworm Spodoptera frugiperda<br />
perceived herbivory through inceptins, a proteolytic fragments of chloroplastic ATP<br />
synthase γ-subunit regulatory regions (Schmelz et al., 2006). Inceptins (feasibly the<br />
receptor molecule) induced volatile, phenylpropanoid <strong>and</strong> protease inhibitor<br />
defenses in cowpea, against fall armyworm. It was also noted that S. frugiperda<br />
larvae having previously ingested chloroplastic ATP synthase γ-subunit proteins<br />
induced cowpea defenses after herbivory.<br />
5.3. Defense Genes in Plants<br />
Intracellular levels of free linoleic <strong>and</strong> linolenic acids increased in tomato leaves on<br />
wounding (Conconi, Miquel, Browse, & Ryan, 1996). The intracellular signalling
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FARHA-REHMAN ET AL.<br />
pathway for activating plant defense genes against attacking herbivores <strong>and</strong><br />
pathogens is mediated <strong>by</strong> a lipid based signal transduction cascade. In this pathway,<br />
linolenic acid (18:3) is liberated from cell membranes <strong>and</strong> is converted to<br />
cyclopentanones involved in transcriptional regulation of plant defense genes<br />
(Conconi et al., 1996).<br />
A wide range of genes in plants are activated on herbivore attacks, <strong>and</strong> their<br />
activation is strongly correlated with the mode of herbivores feeding <strong>and</strong> degree of<br />
tissue damage at the feeding site (Walling, 2000). Phloem feeding whiteflies <strong>and</strong><br />
aphids producing little injury to plant foliage were perceived as pathogens <strong>and</strong><br />
activate the salicylic acid (SA)-dependent <strong>and</strong> JA ethylene-dependent signalling<br />
pathways. Volatiles blends provided specific cues to attract specialist parasites <strong>and</strong><br />
predators to attack infesting herbivores (Walling, 2000).<br />
Herbivory on lima bean leaves induced volatiles elicitor defence genes<br />
(Arimura et al., 2000). In uninfested lima bean leaves, five separate sets of defense<br />
genes were activated on exposure to volatiles from co-specific leaves infested <strong>by</strong><br />
Tetranychus urticae. All these genes were not activated when uninfested leaves were<br />
exposed to volatiles from artificially wounded leaves (Arimura et al., 2000). The<br />
expression pattern of these genes was similar to that produced on exposure to JA. At<br />
least three terpenoids of the released volatiles were responsible for the gene<br />
activation, which were released in response to herbivory but not on artificial<br />
wounding. Expression of these genes required calcium influx <strong>and</strong> protein<br />
phosphorylation/dephosphorylation (Arimura et al., 2000).<br />
The herbivore induced volatiles in Arabidopsis thaliana attracted the parasitoid<br />
Cotesia robecula (Van Poecke, Posthumus, & Dicke, 2001). The A. thaliana plants<br />
infested <strong>by</strong> Pieris rapae emitted volatiles from several major biosynthetic pathways,<br />
including terpenoids <strong>and</strong> green leaf volatiles. Haq et al. (2004) focused on the utility of<br />
the protein proteinase inhibitor genes in combating insects, pests, <strong>and</strong> pathogen as<br />
natural <strong>and</strong> engineered phytoprotection. Devoto et al. (2005) found COII as a key<br />
regulator of genes involved in wound. The methyl jasmonate induced secondary<br />
metabolism, defence <strong>and</strong> hormone interactions. COII expressed approximately 84% of<br />
212 genes induced <strong>by</strong> JA, <strong>and</strong> approximately 44% of 153 genes induced <strong>by</strong> wounding.<br />
COII displayed a pivotal role in wound <strong>and</strong> JA signalling (Devoto et al., 2005). The<br />
volatile emission on green leaf wounding induced the release of acetylated derivatives<br />
<strong>and</strong> a terpenoid in maize, <strong>and</strong> these compounds in turn induced JA production in intact<br />
plants (Yan & Wang, 2006). The wound-induced green leaf volatiles (GLVs) caused<br />
the release of acetylated derivatives <strong>and</strong> a terpenoid, (E)-4,8-dimethylnona-1, 3, 3-<br />
triene (DMNT) in intact maize, which may be a type of plant-plant interaction<br />
mediated <strong>by</strong> airborne GLVs (Yan & Wang, 2006).<br />
Karban <strong>and</strong> Niiho (1995) worked on plant “memory” to induce resistance <strong>and</strong><br />
susceptibility to herbivory. Many plants have been found to be highly induced <strong>by</strong><br />
repeated herbivory, than <strong>by</strong> a single herbivore bout. The frequency <strong>and</strong> magnitude of<br />
damage were confounded <strong>and</strong> thus it was not clear if a biochemical “memory” was<br />
involved or overall damage amplified the induced response (Karban & Niiho, 1995). In<br />
this experiment, the cotton plant attacked <strong>by</strong> spider mites <strong>and</strong> mechanical damage of<br />
cotyledon induced resistance, but damage of apical buds induced susceptibility, due to<br />
differentially affected hormonal regulation in both tissue types (Karban & Niiho, 1995).
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201<br />
Van Poecke, Roosjen, Pumarino, <strong>and</strong> Dicke (2003) noted that different kind<br />
of herbivores induced different signal transduction pathways in A. thaliana. The<br />
varying blends of volatiles were recognized <strong>by</strong> specialist parasitoid (Cotesia<br />
rebecula) of host <strong>and</strong> non-host herbivores.<br />
5.4. Tri-Trophic Plant Signalling<br />
In many plants, Thaler (1999b) found that defence systems against herbivores were<br />
induced through the octadecanoid pathway, which in turn recruited natural enemies<br />
(predators or parasites) of herbivores. This pathway was induceable <strong>by</strong> treating<br />
plants with JA or <strong>by</strong> natural herbivory, as noted in case of tomato plants under insect<br />
herbivory. The plants induced with JA increased parasitism of caterpillar pests in an<br />
agricultural field (Thaler, 1999b). Either JA or herbivory induced carnivores<br />
attraction towards herbivores in lima bean plants (Dicke, Gols, Ludeking,<br />
Posthumus, 1999). Lima bean plants herbivory damage <strong>by</strong> the two spotted spider mite<br />
(Tetranychus urticae) led to the emission of complex blend of volatiles. These volatiles<br />
attracted the carnivorous mite Phytoseiulus persimilis, a specialist predator of spider<br />
mites which exterminated entire population of spider mites. Dicke et al. (1999)<br />
inferred that induction of volatile synthesis in Lima bean plants is almost similar<br />
either caused <strong>by</strong> JA treatment or herbivorous spider mites.<br />
Maize plants (var. LG11) under insect attack released large quantities of volatile<br />
compounds <strong>and</strong> invited parasitic wasps to attack the herbivore (Pare et al., 1998).<br />
Volicitin <strong>and</strong> an elicitor of plant volatile were isolated from beet army worm<br />
caterpillars, <strong>and</strong> were regarded as key components inducing plants to recognize<br />
damage caused <strong>by</strong> herbivory (Pare, Alborn, & Tumlinson, 1998).<br />
Figure 1. Choroedocus illustris feeding on young leaves of Zea mays.
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FARHA-REHMAN ET AL.<br />
Thaler, Farag, Parepaul, <strong>and</strong> dicke (2002) found that jasmonate deficient plants<br />
reduced direct <strong>and</strong> indirect defenses against herbivores. Some plant species had<br />
negative effects on herbivores whereas others had indirect defense against herbivory,<br />
via invitation to the natural enemies of herbivores. It was also noted that damaged<br />
wild type plant were more attractive to predator mites compared with undamaged<br />
wild plant. In both cases, JA is reported to be an essential regulatory component for<br />
the expression of direct <strong>and</strong> indirect plant defences against herbivory (Thaler et al.,<br />
2002). Van Poecke <strong>and</strong> Dicke (2004) reported that Arabiodopsis thaliana defends itself<br />
from pathogens, herbivorous insects <strong>and</strong> mites through induced volatiles emissions, upon<br />
herbivory. These volatiles guided predators or parasites to reach their herbivorous prey,<br />
with a benefit for both the plants <strong>and</strong> the carnivores. Similar indirect defense<br />
patterns have also been noted in pine, maize <strong>and</strong> lima bean.<br />
Figure 2. Choroedocus illustris attacking male inflorescence of Zea mays.<br />
The proline accumulating leaves are preferred <strong>by</strong> grasshoppers. Herbivory<br />
increased the population of grasshoppers in drought stressed plants (Haglund, 1980).<br />
Treatments with low levels of methyl jasmonate resulted in the accumulation of
HERBIVORY & PLANT DEFENSE<br />
203<br />
certain vegetative storage proteins in soybean seedlings, within 3 days of exposure.<br />
The protein accumulated preferably on shoot tips <strong>and</strong> primary leaf. Accumulation of<br />
some specific protein in response to methyl jasmonate was also noticed in<br />
cotyledons. It was inferred that volatile methyl jasmonate acts as gaseous messenger<br />
<strong>and</strong> growth regulator in plants, which alter the nitrogen partitioning (Franceschi &<br />
Grimes, 1991).<br />
In a recent study on maize, the grasshopper Choroedocus illustris attacked<br />
almost every part of the plant. The grasshoppers preferred young leaves mainly in<br />
the apical portion (Fig. 1a, b), <strong>and</strong> also male inflorescence (Fig. 2).<br />
CONCLUSIONS<br />
It is evident from the present review that insects <strong>and</strong> plant co-evolved <strong>and</strong> developed<br />
well defined mechanisms to regulate the uptake of a limited amount of plant <strong>org</strong>anic<br />
matter to higher trophic levels. In this review emphasis has been given to underst<strong>and</strong><br />
the natural mechanism of control over herbivore consumption <strong>and</strong> the way in which<br />
energy is transferred from primary producers to the <strong>org</strong>anisms of higher trophic<br />
levels. Plant <strong>and</strong> insects co-evolution allows the onset of a balanced primary<br />
productivity, which is partitioned to the second trophic level <strong>and</strong> beyond. During<br />
their course of evolution, plants not only developed morphological defense<br />
mechanisms active against insect herbivory, but also genetic transformations<br />
allowing the production of volatile chemicals. Attacked plants use these volatile<br />
chemicals as arsenals <strong>and</strong> signals against attacking pests. These chemicals not only<br />
repell herbivores but also control their population, <strong>by</strong> signalling invitations sent to<br />
their predators or parasites. For all these purposes plants synthesize special blends of<br />
volatile chemicals only after insect attack. The interaction between herbivores <strong>and</strong><br />
biotic environment is thus largely based on plant mediated mechanisms, including<br />
constitutive traits like modifications in plants anatomy <strong>and</strong> physiology, or herbivore<br />
induced changes in host biochemistry (Elliot, Sabelis, Janssen, Van der Geest, &<br />
Berling, 2000; Ode, 2006; Ohgushi, 2005; Price et al., 1980). The plant mediated<br />
interactions can furthermore operate among spatially <strong>and</strong> temporally separated<br />
<strong>org</strong>anisms, even at low herbivory levels (Ohgushi, 2005).<br />
The energy cost – benefit ratio between crop losses <strong>and</strong> pesticides use show that<br />
about 50% of losses are due to pests. Under natural conditions, the energy transfer<br />
from plants to herbivores has a far lower magnitude (Kormondy, 2003), even<br />
without use of pesticides. These compounds have in the ecosystem a far reaching<br />
impact, <strong>and</strong> may eliminate herbivores predators from the ecosystem. Thus, within a<br />
single crop cycle, the natural process of controlled biomass transfer from one trophic<br />
level to the higher one may be altered, in a structural way. If the process of plant<br />
signalling is activated <strong>and</strong> applied, it may prove to be more effective than pesticides<br />
in maintaining stable populations of plants, herbivores <strong>and</strong> predators.<br />
Plants also evolved direct strategies to repel herbivores, through induced <strong>and</strong><br />
constitutive defence mechanism. The trichomes constitute a defense feature against a<br />
variety of insects. But plants also evolved mechanisms based on volatile substances<br />
acting during insect attacks that, on one h<strong>and</strong> repell an attacking insect directly,
204<br />
FARHA-REHMAN ET AL.<br />
whereas on the other h<strong>and</strong> invite its predators. This mechanism becomes operational<br />
only on herbivore attack. The reaction of herbivores oral secretion <strong>and</strong> plant elicitors<br />
activates certain host genes. Thus, plants rely on a system of multiple chemical<br />
switches that control the partitioning of biomass to herbivores <strong>and</strong> predators, at least<br />
up to three trophic levels. Moreover, plants have either no or limited “memory” of<br />
previous insect attack, with some exceptions. Thus, an equilibrium in the transfer of<br />
biomass from hosts to herbivore-predators is maintained naturally, throughout the<br />
plants life cycle.<br />
Among pests response to plants arsenals, it is worth to recall how herbivorous<br />
insects evolved adaptive mechanism to search suitable healthy plants for oviposition.<br />
As shown, nocturnal pests, i.e. Heliothis veriscence avoid injured plants during day<br />
time for oviposition, to save their offsprings from day time predators (De Moraes<br />
et al., 2001).<br />
Herbivory caused <strong>by</strong> grasshoppers accelerated nutrients cycling <strong>and</strong> plant<br />
production <strong>and</strong> abundance (Belovsky & Slade, 2000). It is also reported that larvae<br />
of M<strong>and</strong>uca sexta modified, before feeding on damage leaves, the host normal<br />
defensive metabolites <strong>by</strong> reducing systemic JA in roots, <strong>and</strong> subsequently the<br />
nicotine content in the whole plant (McCloud & Baldwin, 1997).<br />
Herbivores <strong>and</strong> predators also rely on receptor molecules, starting from the<br />
activation of plants defense genes on an insect attack. Plant defences to herbivory<br />
can be simulated <strong>by</strong> JA, since in some plants the defense mechanism was brought<br />
under operation through JA <strong>and</strong> artificial injury together. However, more<br />
experiments are required to induce chemical defense <strong>and</strong> use this mechanism of<br />
chemical signalling for pests control, in a way that may be much more effective <strong>and</strong><br />
environment friendly than using pesticides. Biological control may prove indeed to<br />
be more economic not only for crop losses, but also for the ecosystem maintenance.<br />
It must be kept in mind that elimination of one herbivore species may prove to be<br />
more detrimental for the ecosystem if it happens to be a keystone species. Any<br />
biological control strategy should seek at an equilibrium among plant biomass,<br />
herbivores as well as predator populations, to be maintained<br />
Plants adaptive mechanism evolved to ward off herbivores is both structural <strong>and</strong><br />
functional (constitutive <strong>and</strong> inducible). Host plants synthesize volatile chemicals as<br />
part of their defense strategies against excessive herbivory. Artificial injury induced<br />
<strong>by</strong> leaf clipping in some species did not produce the blend of volatiles which are<br />
repulsive for herbivore or provide clues to the predators, since they possess specific<br />
genes activating the synthesis of volatiles only on an insect attack <strong>and</strong> up regulated<br />
<strong>by</strong> the chemicals contained in the herbivores mouth.<br />
The volatiles synthesized in plant tissues after insects attack were useful to ward<br />
off insect directly. Also, since the volatiles provide clues to the predator about<br />
the preys (herbivores) presence <strong>and</strong> also signal the neighbouring undamaged plants about<br />
the attack of the herbivores, the course of co-evolution acquired a higher level of<br />
complexity when certain insect species cleverly adopted to these volatiles. Some<br />
herbivores, furthermore, were capable to modify the blends of volatiles <strong>and</strong> thus<br />
used modified plant arsenals (volatiles) to defend themselves from the predator.<br />
Due to co-evolution, most plants had limited memory for insect attack but not in<br />
some perennial trees (mainly Australian eucalypts), in which the plant volatiles were
HERBIVORY & PLANT DEFENSE<br />
205<br />
synthesized for longer duration <strong>and</strong> controlled insect population. Similarly, due to<br />
the adaptation of herbivores to modify the blends of chemicals, the role of plant<br />
volatiles in inviting predators or parasites results in an ecosystem-wide effect,<br />
influencing the flow of material <strong>and</strong> energy along the trophic level, as well as the<br />
population equilibrium levels, at each trophic level. Due to co-evolution of synthesis<br />
of herbivore repelling volatiles in plants <strong>and</strong> their modification <strong>by</strong> herbivores, cyclic<br />
population changes, concerning both the herbivores <strong>and</strong> primary producers, can also<br />
be affected. This aspect needs attention <strong>and</strong> attempts to increase the amount of data<br />
through further studies <strong>and</strong> may prove useful in biological control of crop herbivory.<br />
ACKNOWLEDGEMENTS<br />
Authors acknowledge the Departments of Botany <strong>and</strong> Zoology, Aligarh Muslim<br />
University for necessary facilities, <strong>and</strong> funding agencies for financial assistance.<br />
Farha-Rehman acknowledges U.G.C. for research fellowship. S.M.A. Badruddin<br />
thanks ICAR for funding through the “Network Project on Insect Biosystematics”.<br />
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9<br />
IPM OF THE RED PALM WEEVIL,<br />
RHYNCHOPHORUS FERRUGINEUS<br />
MOHAMED SAMIR TAWFIK ABBAS<br />
Plant Protection Research Institute,<br />
Dokki, Cairo, Egypt<br />
Abstract. The Red Palm Weevil (RPW) Rhynchophorus ferrugineus is the major destructive insect<br />
pest of a broad range of palm trees. Infestation <strong>by</strong> RPW varies in relation to the height <strong>and</strong> age of<br />
palm trees <strong>and</strong> most likely is restricted to 0–1 m height above soil surface <strong>and</strong> to palms up to 10<br />
years old. The life cycle of the insect in the laboratory may last several months depending on the<br />
type of food, temperature as well as the procedure of rearing. A single female may produce more<br />
than 400 eggs during its life-time, which may last more than 6 months. Natural enemies recorded for<br />
RPW include parasitoids, predators <strong>and</strong> insect pathogens (bacteria, viruses, fungi <strong>and</strong> nematodes).<br />
However, such recorded natural enemies do not have considerable role against the insect. Chemical<br />
control with different insecticides was applied against the insect as spraying, trunk injection as well<br />
as fumigation, with phostoxin tablets. Alternative safe methods of control were investigated using<br />
entomopathogenic nematodes, fungi or aggregation pheromone traps. The latter proved to be a<br />
promising means of control against this insect.<br />
1. INTRODUCTION<br />
The Red Palm Weevil (RPW), Rhynchophorus ferrugineus (Coleoptera:<br />
Curculionidae) is the major destructive insect pest of a broad range of palms<br />
including date, coconut, sago, oil palm, toddy <strong>and</strong> royal palm (Nirula, 1956). It<br />
was first recorded in 1889 in India as the most deadly insect pest of the coconut<br />
palms (Leefmans, 1920). The insect was later recorded in Ceylon <strong>and</strong><br />
Philippines in 1906, Indonesia in 1920 (Nirula, 1956) <strong>and</strong> later detected in the<br />
Gulf area in mid 1980s, the United Arab Emirates (UAE) in 1985 (FAO, 1995),<br />
Saudi Arabia in 1986, Qatar in 1989 (Abdulla, 1997), the Sultanate of Oman in<br />
1993 (Al-Kaabi, 1993), Kuwait in 1993 (FAO, 1995), Bahrain in 1995 (Hamdi,<br />
1998) <strong>and</strong> Iran in 1992. The insect was able to cross the Red Sea as it was then<br />
found in Egypt in 1992 (Cox, 1993) <strong>and</strong> in Palestine, Israel <strong>and</strong> Jordan in 1999<br />
(Kehat, 1999). It was also able to cross the Mediterranean Sea to become a<br />
serious pest in Spain, France, <strong>Italy</strong> <strong>and</strong> Greece (Manachini, Mansueto, Arizza, &<br />
Parrinello, 2008).<br />
209<br />
A. <strong>Ciancio</strong>, K.G. Mukerji (eds.), Integrated Management of Arthropod Pests<br />
<strong>and</strong> Insect Borne Diseases, Integrated Management of Plant Pests <strong>and</strong> Diseases 5,<br />
DOI 10.1007/978-90-481-8606-8_9, © Springer Science+Business Media B.V. 2010
210<br />
M.S.T. ABBAS<br />
The high rate of spread of this pest is due to the human intervention, <strong>by</strong><br />
transporting infested young date palm trees <strong>and</strong> offshoots from infested to<br />
healthy areas <strong>and</strong> countries. For example, the insect invaded Egypt when<br />
infested offshoots were imported from UAE in November 1992 (Cox, 1993).<br />
Also, as reported <strong>by</strong> Ferry <strong>and</strong> Gomez (2002), there was evidence suggesting<br />
that the first weevils were introduced into Spain from adult palms imported from<br />
Egypt.<br />
Leefmans (1920) published the first original investigation on the pest in<br />
Indonesia, <strong>and</strong> gave a complete description of the pest suggesting various<br />
control measures.<br />
2. HABITAT, INFESTATION AND DAMAGE<br />
The crown <strong>and</strong> trunk of the palm tree represent the natural habitats of all stages<br />
of R. ferrugineus. In old coconut palms the infestation is restricted to the crown,<br />
while in young trees of coconut <strong>and</strong> date palms it is present in the crown but<br />
mainly in the trunk. More often the insect resides in the trunk where it passes<br />
many generations, feeding into the soft tissue portions until the trunk is<br />
completely hollowed out <strong>and</strong> the tree falls down. The early symptom of RPW<br />
infestation is a brown <strong>and</strong> bad smelling sap exudated from the point of<br />
infestation. However, such a symptom could be invisible, especially when<br />
infestations occur at the base of the trunk.<br />
The infestation <strong>by</strong> RPW varies in relation to the height <strong>and</strong> age of the date<br />
palm trees. In a study in Saudi Arabia 50% of infestations occurred at heights<br />
between 0 <strong>and</strong> 1 m from the trunk base, whereas 38% was within 1–2 m<br />
(Anonymous, 2001). As for the age of palms, most of infestation was found in<br />
palms 5–10 years old, while prevalence was lower in palms older than 15 years.<br />
In a similar study in UAE, Khalifa et al. (2007) reported percentages of<br />
RPW infestation in different date palm plantations as 77.8% at 0–50 cm <strong>and</strong><br />
20.4% at 51–100 cm (total prevalence was 98.2% within 0–1 m). No infestation<br />
could be detected at heights higher than 3 m. Similarly, prevalence was 12.8% at<br />
ages up to 5 years <strong>and</strong> gradually increased to 64.8% at 6–10 years of age. The<br />
infestation was noticed to decrease gradually to reach 17.1, 3.3 <strong>and</strong> 1.3% at ages<br />
of 11–15, 16–20 <strong>and</strong> >20 years, respectively. However, in Egypt, in old palms<br />
some infestations were found at the heights around 6 m, so that the palms were<br />
broken at that level (unpublished). This case was attributed to the fact that RPW<br />
infestation occurred at the crown of palm <strong>and</strong> the larvae moved, in tunnels,<br />
downward until the tree collapsed at that height.<br />
2.1. Infestation Spreading<br />
Once RPW is introduced into an area or even a country, it has great ability to<br />
disperse <strong>and</strong> exp<strong>and</strong>. For example, R. ferrugineus was introduced for the first<br />
time in Egypt through imported offshoots transplanted in two close locations in<br />
Sharkyia governorate, northeastern of Cairo (Cox, 1993). Since then, great
IPM OF RED PALM WEEVIL<br />
211<br />
efforts have been done to eradicate the insect using intensive spraying of<br />
chemical insecticides in both locations, mass trapping <strong>by</strong> pheromone traps as<br />
well as <strong>by</strong> cutting, burning <strong>and</strong> burying the infested palm trees. In 1995, despite<br />
these efforts, a RPW infestation was detected in Ismailia governorate (50 km<br />
apart from initial focus) <strong>and</strong> later, in the following years, the insect spread in<br />
most governorates in Egypt. This extensive spread is certainly due partly to: (i)<br />
the exchange <strong>and</strong> transplanting of offshoots <strong>and</strong> ornamental adult palms, (ii) the<br />
partial burning of trunks which did not kill all insects inside such palms <strong>and</strong> (iii)<br />
superficial burying of burned palms, that allowed the formed RPW adults to<br />
emerge from soil for months.<br />
Another example was reported <strong>by</strong> Gomez Vives <strong>and</strong> Ferry (1999) who<br />
mentioned that in Spain very soon after RPW killed the first Phoenix canariensis<br />
in some gardens at Almufiecar, intensive chemical treatments were applied to<br />
affected trees. Foliage spraying was conducted with various insecticides <strong>and</strong><br />
preventive treatment of all palms, even healthy ones, was repeated once a month.<br />
Simultaneously, a mass trapping program using aggregation pheromone was<br />
initiated. However, despite all such efforts, more than one thous<strong>and</strong> plants were<br />
killed <strong>and</strong> the area of infestation exp<strong>and</strong>ed to villages close to the initial focus.<br />
3.1. Morphological Characters<br />
3. BIOLOGY<br />
RPW male <strong>and</strong> female adults are large reddish-brown weevils about 3 cm long<br />
with a long curved rostrum. They are capable of flying to long distances. The<br />
egg is creamy-white, long oval in shape, smooth <strong>and</strong> shiny. It is about 2.5 mm<br />
long <strong>and</strong> 1.1 mm wide. The full-grown larva (13 segments) is a conical shaped,<br />
plugged in the middle <strong>and</strong> pointed towards both ends with no legs. The head is<br />
light brown with well-developed mouth parts. The average length of the full<br />
grown larva is 50 mm with an average of 20 mm in width. The newly formed<br />
pupa is creamy in color <strong>and</strong> turns brown gradually. It is almost 35 mm long <strong>and</strong><br />
15 mm wide. The cocoon, constructed from palm tissues, is oval in shape, light<br />
brown in color, in average of 60 mm long <strong>and</strong> 30 mm wide (Fig. 1).<br />
3.2. Life Cycle<br />
The life cycle of RPW was investigated <strong>by</strong> many authors. In the laboratory, the<br />
durations of the immature stages, adult longevity, total number of eggs<br />
deposited <strong>by</strong> a single female <strong>and</strong> sex ratio varied, as shown in Table 1. Such<br />
variations could be attributed to the rearing facilities <strong>and</strong> the food substrate for<br />
the larvae <strong>and</strong> adults.<br />
3.2.1. Oviposition<br />
The female starts oviposition 2–11 days after emergence from cocoons, in the<br />
softer portion of the palm in which they feed (Nirula, 1956). It was believed that<br />
RPW attacks only the palms which have been injured <strong>by</strong> the beetle Oryctes
212<br />
M.S.T. ABBAS<br />
rhinoceros but it has been proved that the weevil attacks healthy <strong>and</strong> uninfested<br />
palms (personal observations). To oviposit, the female uses the rostrum to bore<br />
into the tissues, mainly under the leaf base, to form a hole in which the eggs are<br />
laid, then the hole is cemented to protect them from natural enemies.<br />
Figure 1. Life cycle of the Red Palm weevil, Rhynchophorus ferrugineus.<br />
3.2.2. Feeding<br />
RPWs feeding takes place on the soft portions of the palm. In the field, the<br />
weevils select a suitable site with the help of their antennae <strong>and</strong> thrust in their<br />
long rostrum at that spot, to feed on the juice. The feeding scars are quite<br />
superficial <strong>and</strong> can be readily differentiated from the oviposition holes which are<br />
deeper (Nirula, 1956). In the laboratory, when weevils feed on pieces of sugarcane<br />
or palms it was noticed that they grind such blocks <strong>by</strong> their mouth parts,<br />
sucking the juice <strong>and</strong> discarding the remains as ground material (personal<br />
observations).
IPM OF RED PALM WEEVIL 213
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M.S.T. ABBAS<br />
3.2.3. Locomotion<br />
Flight of the weevils is restricted to day time <strong>and</strong> they have never been observed<br />
as attracted <strong>by</strong> light traps (Nirula, 1956). Al-Khatri <strong>and</strong> Abd-Allah (2003)<br />
studied the daily active periods of R. ferrugineus in date palm plantations in<br />
Oman, using the pheromone traps. They found that the weevils had two periods<br />
of activity, the first between 6 <strong>and</strong> 9 am <strong>and</strong> the second between 6 <strong>and</strong> 9 pm<br />
(sunrise in that area during the period of the study was at 6:15 am <strong>and</strong> sunset<br />
was at 5:50 pm). The weevils were noticed to have no activity during the periods<br />
between 9 am <strong>and</strong> 3 pm <strong>and</strong> between midnight to 3 am. Similarly, Gunawardena<br />
<strong>and</strong> B<strong>and</strong>arage (1995) reported that the periods of RPW activity in Sri Lanka<br />
were between 6 <strong>and</strong> 8 am <strong>and</strong> between 6 <strong>and</strong> 8 pm.<br />
RPW adults are capable of flying as well as crawling. When they are thrown<br />
in the air they fly away in a circle with a buzzing noise <strong>and</strong> quickly disappear,<br />
sometimes l<strong>and</strong>ing shortly <strong>and</strong> boring into the soil. It is believed that the insect<br />
is capable of either flying to a long distance or being carried <strong>by</strong> the winds. It was<br />
noticed that when a weevil was attracted to a pheromone trap it l<strong>and</strong>ed at less<br />
than 1 m apart from the trap, then crawled until reaching it (personal<br />
observation). Chinchilla, Oehlschlager, <strong>and</strong> Gonzaler (1993) reported that the<br />
average flight of R. ferrugineus adults was around 500 m per day <strong>and</strong> a small<br />
portion of the insect migrated up to 1 km per day. Abbas, Hanounik, Shahdad,<br />
<strong>and</strong> Al-Bogham (2006) found that when marked RPWs were released in date<br />
palm plantations, some of them were captured <strong>by</strong> pheromone traps in other<br />
plantations, 1–7 km apart from the release area. Most of such weevils were<br />
captured 3–5 days post release.<br />
4. NATURAL ENEMIES<br />
There are few records about the occurrence of natural enemies of R. ferrugineus,<br />
which might be attributed to the cryptic habitat of the eggs, larvae <strong>and</strong> pupae<br />
which protects them from such natural enemies.<br />
4.1. Parasitoids<br />
Scolia erratica (Hym.: Scoliidae) was reported as an ectoparasitoid of R. ferrugineus<br />
larvae (Nirula, 1956). However, no biological studies on this parasitoid have<br />
been reported. In Brazil, Moura, Mariau, <strong>and</strong> Delabie (1993) <strong>and</strong> Moura,<br />
Resende, <strong>and</strong> Vilela (1995) reported the tachinid Paratheresia menezesi as a<br />
larval-pupal parasitoid of R. palmarum <strong>and</strong> many individuals of the parasitoid<br />
adults emerged from a single pupa. However, attempts were carried out to rear<br />
this parasitoid on R. ferrugineus in the laboratory, but the results were<br />
unsuccessful (unpublished). Nirula (1956) mentioned that both RPW pupae <strong>and</strong><br />
adults were attacked <strong>by</strong> an unknown species of parasitic mite which killed the<br />
pupae <strong>and</strong> reduced the longevity of adults.
IPM OF RED PALM WEEVIL<br />
215<br />
Peter (1989) recorded two mite species, Hypoaspis sp. <strong>and</strong> Tetrapolypus<br />
rhynchophori (Pymotidae) parasitizing the RPW adults <strong>and</strong> mentioned that the<br />
status of such mites as parasitoids was uncertain.<br />
4.2. Predators<br />
Although the earwigs (Forficulidae: Dermaptera) are considered scavengers,<br />
Abraham, Kurian, <strong>and</strong> Nayer (1973) recorded Chelisoches morio as a common<br />
predator inhabiting the crown of coconuts in Kerala, India. The authors<br />
mentioned that the daily average consumption <strong>by</strong> nymphs <strong>and</strong> adults of the<br />
predator varied between 5.3 <strong>and</strong> 8.5 R. ferrugineus eggs, or 4.2 <strong>and</strong> 6.7 larvae,<br />
respectively. In Saudi Arabia, the earwig, Anisolabis maritima <strong>and</strong> the<br />
anthocorid, Xylocorus galactinus were recorded as common predators on RPW<br />
eggs, larvae <strong>and</strong> pupae (Anonymous, 2001).<br />
Anisolabis maritima, showed a higher predatory efficiency. An assay was<br />
carried out in Saudi Arabia to evaluate its efficiency as a biocontrol agent<br />
against R. ferrugineus, on 5 year old date palm offshoots (each caged in a wirecage,<br />
2 × 2 × 2 m). Three pairs of RPW were introduced in each cage in which<br />
A. maritima was released after 24 h, at rates of 5, 10, 15 <strong>and</strong> 20 pairs per<br />
offshoot. One month later, 50% of the offshoots were dissected <strong>and</strong> the numbers<br />
of RPW larvae were recorded. The results showed that percentages of infestation<br />
in the treated offshoots were 50% (in offshoots with 5 predator couples), 25%<br />
(in offshoots with 10, 15 or 20 couples) <strong>and</strong> 100% (control). A significant<br />
reduction in the numbers of RPW larvae was obtained in the offshoots with<br />
predators, compared to the control. The larvae found in the five treatments were<br />
12% (in offshoots with 5 or 10 couples), 28% (in offshoots with 15 pairs), 4%<br />
(in offshoots with 20 pairs) <strong>and</strong> 44% (control) (Anonymous, 2001).<br />
The duration of the immature stages of X. galactinus were estimated when<br />
fed on eggs, 1st instar larvae or pupae of R. ferrugineus in the laboratory at 25°C<br />
in Saudi Arabia. It was found that the incubation period of the predator egg was<br />
3.6 days (3–4). The nymph (5 instars) lasted 16.5 days (14–19) when fed on 1st<br />
instar larvae <strong>and</strong> 15.5 days (14–17) when feeding on RPW pupae. The average<br />
daily consumption of a X. galactinus nymph was 1.2–1.8 eggs or 3 larvae. The<br />
adult consumed 1.8–2 eggs or 3.6 larvae, daily (Anonymous, 2001).<br />
Xylocorus galactinus was also obtained <strong>by</strong> M.S.T. Abbas (unpublished) in<br />
Egypt from a fallen date palm tree, severely infested. However, this species was<br />
found associated with larvae of the house fly, Musca domestica, feeding on the<br />
fermented decayed tissues of such a tree. In a food preference test, <strong>by</strong> exposing<br />
larvae of M. domestica together with eggs <strong>and</strong> 1st instar larvae of R. ferrugineus,<br />
the predator attacked <strong>and</strong> consumed only larvae of M. domestica. In agreement<br />
with this finding, Tawfik <strong>and</strong> El-Husseini (1971) recorded X. galactinus as a<br />
predator of M. domestica inhabiting <strong>org</strong>anic manure <strong>and</strong> animal’s dung.<br />
4.3. Pathogens<br />
Banerjee <strong>and</strong> Dangar (1995) isolated the bacterium Pseudomonas aeruginosa<br />
from naturally infected adults of R. ferrugineus in Kerala, India. The bacterium
216<br />
M.S.T. ABBAS<br />
was found to be pathogenic to adults forced to feed on a suspension of bacterial<br />
cells, <strong>and</strong> mortality occurred 8 days after ingestion.<br />
In India, a highly potent cytoplasmic polyhedrosis virus (CPV) specific to<br />
RPW was also found (Gopinadhan, Moh<strong>and</strong>as, & Nair, 1990). The virus<br />
infected all stages of the insect <strong>and</strong> laboratory infection of late larval stages<br />
resulted in the development of malformed adults.<br />
Among fungi, Beauveria bassiana was isolated from adults of R. ferrugineus<br />
in UAE <strong>and</strong> Saudi Arabia, through a project operated <strong>by</strong> the Arab Organization<br />
for Agriculture Development (AOAD), in the period 1997–2007 (Anonymous,<br />
2008). The fungus was found to be highly pathogenic to both larvae <strong>and</strong> adults<br />
in the laboratory (Hanounik et al., 2000b; El-Safty et al., 2007).<br />
4.4. Nematodes<br />
Praecocilenchus ferruginophorus (Aphelenchida) was recorded parasitizing R.<br />
ferrugineus adults in India (Rao & Reddy, 1980). The size of the nematodes<br />
found in the haemocoel ranged from small intrauterine specimens to larger<br />
mature parasitic females, suggesting several simultaneous <strong>and</strong> unsynchronized<br />
life cycles in the weevils. Abbas, Hanounik, Mousa, <strong>and</strong> Awash (2001b) <strong>and</strong><br />
Abbas, Hanounik, Mousa, <strong>and</strong> Mansour (2001c) isolated two entomopathogenic<br />
nematodes (EPN), namely Steinernema abbasi <strong>and</strong> Heterorhabditis indicus from<br />
adult R. ferrugineus. They also showed that 20–100% of the RPW adults were<br />
found hosting other non pathogenic, unidentified nematodes.<br />
5.1. Chemicals<br />
5.1.1. Spraying<br />
5. CONTROL<br />
Preventative <strong>and</strong> curative spraying of chemical insecticides have been the most<br />
common method applied for RPW control. All groups of insecticides have been<br />
tested <strong>and</strong> applied as foliage <strong>and</strong> trunk sprayings. For example, Soenardi <strong>and</strong><br />
Hariadi (1978) reported that application of sevin or carbaryl gave effective field<br />
control when applied every 2 months. Also, Abraham, Koya, <strong>and</strong> Kurian (1975)<br />
tested seven insecticides against R. ferrugineus in Kerala, India <strong>and</strong> found that<br />
trichlorphon gave the best control, with 92% of the infested palms recovering<br />
from weevil infestation. In Egypt, El-Sebaey (2004a), concluded after field trials<br />
that offshoots could be protected from RPW infestation for 11–13 weeks, <strong>by</strong><br />
dipping them for 15 min in a mixture of the insecticides confidor (75 ml/100 l of<br />
water), oshin (125 g/100 l) mixed with 250 g/l of mud, before translocation <strong>and</strong><br />
re-cultivation.<br />
It was observed that many infested trunk bases of date palms harbored<br />
reliable numbers of different alive stages of RPW, below the soil surface. Such<br />
trunk bases last alive, after removing severely infested palms above the ground
IPM OF RED PALM WEEVIL<br />
217<br />
level, for a long time (El-Sebaey, 2004a). In this respect, this author carried out<br />
an experiment using chemical insecticides to kill all developmental stages of<br />
RPW surviving in such trunk bases. Big holes were made in the bases, using a<br />
sharp axe, to facilitate penetration of insecticides downward through the base<br />
tissues. Six chemical insecticides, dissolved either in water or kerosene, were<br />
poured at rates ranging from 5 to 10 l/base. Two weeks later, the treated bases<br />
were picked up using a loader machine <strong>and</strong> cut into parts to allow inspection of<br />
alive <strong>and</strong>/or dead RPW stages, inside the base <strong>and</strong> root system. The experiment<br />
showed that the insecticides Cidial (phenthoate), Basudin (diazinone) <strong>and</strong><br />
Dursban (chlorpyrifos-ethyl), dissolved in kerosene, caused 100% mortality in<br />
larvae <strong>and</strong> pupae. As for adult weevils they caused 95.6, 95.2 <strong>and</strong> 97.6%<br />
mortalities, respectively. However, the same insecticides, dissolved in water,<br />
caused 57, 53 <strong>and</strong> 49% mortalities in larvae, 37, 55 <strong>and</strong> 48% mortalities in<br />
pupae, <strong>and</strong> 25, 25 <strong>and</strong> 26% mortalities in adults. The author related the<br />
synergistic action of kerosene to three factors: (i) its function as a good carrier<br />
for the chemicals throughout the wood fibers deeply inside the infested roots,<br />
(ii) its physical action on the wood as a dehydrated substance which caused<br />
wood dryness faster than insect survive, <strong>and</strong> (iii) its effect on dehydration <strong>and</strong><br />
toxic action on the insects' cuticle.<br />
5.1.2. Injection<br />
Injection of insecticides into the trunk of the coconut palm was first reported <strong>by</strong><br />
Rao, Subramaniam, <strong>and</strong> Abraham (1973), who demonstrated that the direct<br />
injection of 0.2% fenthion gave effective control of larvae in the tree.<br />
Muthuraman (1984) reported that 10 ml of monocrotophos or dichlorovos<br />
injected into a pre–drilled 10 cm deep hole above the infestation site gave 100%<br />
recovery of the treated infested trees. In Egypt, El-Sebaey (2004b) tested 15<br />
chemical insecticides against RPW infestation <strong>by</strong> injecting them at different<br />
concentrations in 4–10 holes (10 cm deep), drilled around the infestation site.<br />
This author found that all tested chemicals showed 100% recovery of infestation<br />
at a concentration of 10,000 ppm, while at 100 ppm dursban, curacron <strong>and</strong> cidial<br />
gave 80% recovery.<br />
An alternative to injecting insecticides into the tree is sealing, inside the tree,<br />
a tablet form of a slow release fumigant. Phostoxin tablets (aluminum<br />
phosphide) applied at a rate of 0.5–1 tablet per tree was effective in killing<br />
larvae, pupae <strong>and</strong> adults of RPW on coconut (Rao et al., 1973).<br />
Muthuraman (1984) used two 3 g celphos (aluminum phosphide) tablets<br />
crushed, placed in holes in date palms <strong>and</strong> sealed with a paste of cement <strong>and</strong><br />
copper oxychloride.<br />
Abd-Allah <strong>and</strong> Al-Khatri (2000a) compared the effectiveness of injecting<br />
chemical insecticides <strong>and</strong> using fumigation tablets (aluminum phosphide)<br />
against RPW infestation. In this experiment, three holes (30 cm deep <strong>and</strong> 1.9 cm<br />
wide) were drilled into the tree: one at the point of infestation (where the brown<br />
bad smell sap was oozing), the second 20 cm above <strong>and</strong> the third 20 cm below<br />
the first hole. Into each hole 50 ml of the insecticide formothion 33% was<br />
poured using a plastic tube (45 cm long <strong>and</strong> 1.3 cm diameter). The holes were
218<br />
M.S.T. ABBAS<br />
sealed with moistened clay. In case of fumigation tablets, the part of the trunk<br />
where oozing occurred was cleaned <strong>and</strong> the decaying tissues <strong>and</strong> grubs were<br />
removed as much as possible. One aluminum phosphide tablet (3 g) was placed<br />
in the formed cavity then sealed with moistened clay.<br />
The treated palm trees were inspected at 2-week intervals for 10 weeks. The<br />
experiment showed that injecting formothion in the infested date palms was<br />
much more effective compared to the fumigation tablets. The authors concluded<br />
that aluminum phosphide was not effective in controlling RPW in infested trees.<br />
They attributed this failure to (i) the escape of gas through many crevices in the<br />
tree <strong>and</strong> (ii) the feces <strong>and</strong> frass which, forming a thick paste, block the larval<br />
tunnels so that it is difficult for the gas to diffuse to reach the larvae.<br />
5.2. Aggregation Pheromone Traps<br />
Trapping of palm weevils started with utilizing insecticide – treated palm stems<br />
(Mariau, 1968; Griffith, 1969) followed <strong>by</strong> utilizing treated fruits or sugar-cane<br />
in plastic buckets hung on the trunk at heights of 1–1.5 m (Delgado & Orellana<br />
Moreno, 1986). A male–produced aggregation pheromone was first identified<br />
for R. palmarum <strong>by</strong> Rochat, Gonzales, Mariau, Villanueva, <strong>and</strong> Zagatti (1991a)<br />
<strong>and</strong> Rochat et al. (1991b). Chinchilla et al. (1993) reported that the most<br />
efficient <strong>and</strong> convenient traps for R. palmarum infesting oil palm consisted of<br />
19 l plastic buckets, containing such a pheromone <strong>and</strong> carbofuran-treated<br />
sugarcane.<br />
Hallett et al. (1993) demonstrated that 4-methyl-5-nonanol (ferrugineol) is an<br />
aggregation pheromone to R. ferrugineus <strong>and</strong> R. vulneratus. While another<br />
compound, 4-methyl-5-nonanone (ferrugineone) was found to have bioactivity<br />
only for R. ferrugineus. In field trials, these authors found that R. ferrugineus<br />
was captured in traps with ferrugineol alone or in a 10:1 ratio with<br />
ferrugineone. Increasing amounts of ferrugineone significantly decreased<br />
attraction of R. ferrugineus. Interestingly, they also found that using 10 alive males<br />
of R. ferrugineus in trap instead of ferrugineol <strong>and</strong> ferrugineone (in 10:1 ratio),<br />
was as attractive as the latter for both R. ferrugineus <strong>and</strong> R. vulneratus.<br />
5.2.1. Trap Design <strong>and</strong> Components<br />
Abd-Allah <strong>and</strong> Al-Khatri (2000b) evaluated nine different designs of pheromone<br />
traps (20 l plastic bucket hung on tha palm trunk at a height of 1.7 m), for their<br />
rate of capturing R. ferrugineus adults. They found that the most efficient<br />
pheromone trap was the open one (without a lid) followed <strong>by</strong> the trap with a<br />
plastic lid. The latter had six lateral holes (3 cm in diameter) <strong>and</strong> four similar<br />
holes on the lid. Both traps contained a pack of commercial aggregation<br />
pheromone attached to one side of the bucket. The traps were provided also with<br />
1 kg of dates, 5 g of yeast <strong>and</strong> 5 l of water.<br />
A modification in the trap with a lid was made through a project for RPW<br />
biological control adopted <strong>by</strong> AOAD, carried out in Gulf countries in 1997–2007
IPM OF RED PALM WEEVIL<br />
219<br />
(Anonymous, 2000). A pack of kairomone (synthetic volatile material induced<br />
<strong>by</strong> palm tissues which attracts RPW) is attached beside the pack of the<br />
aggregation pheromone on the inner surface of the lid, to enhance the rate of<br />
capture. Recently, some companies are producing a pack of a mixture of<br />
aggregation pheromone <strong>and</strong> kairomone.<br />
A field trial was carried out to evaluate the rate of catch of the pheromone<br />
plus kairomone traps, compared to those with pheromone only. The trial<br />
revealed that the pheromone plus kairomone traps captured more weevils than<br />
the traps without kairomone. However, the difference in capture rates between<br />
traps was insignificant. Pieces of palm tissues, date fruits or sugar-cane were<br />
considered to have a role in pheromone traps. The catch of R. ferrugineus in<br />
pheromone traps containing the commercial aggregation pheromone <strong>and</strong> dates<br />
was hence compared to the catch in traps containing either the pheromone alone<br />
or dates alone. The numbers of RPW captured in 16 traps during a year were<br />
1,752, 181 <strong>and</strong> 54 insects for the three treatments, respectively (Al-Saoud,<br />
2007). Similarly, Chinchilla et al. (1993) reported that pheromone traps of R.<br />
palmarum captured 6–30 times more weevils than traps containing palm tissues<br />
or sugar-cane alone.<br />
Figure 2. Pheromone terrestrial traps.<br />
5.2.2. Trap Installation<br />
Pheromone traps were reported to be attached or hung close to palm trees at 1–<br />
1.7 m height (Oehlschlager, Chinchilla, & Gonzales, 1992; Chinchilla et al.,<br />
1993; Abd-Allah & Al-Khatri, 2000b). In field trials, rate of catch of RPW was<br />
evaluated in pheromone traps with plastic lids in three date palm plantations<br />
installed at a rate of 1 trap per ha (Anonymous, 2000). In each plantation, 6 traps<br />
were buried in the soil up to the lateral holes below the lid of the trap (terrestrial<br />
traps, Fig. 2) <strong>and</strong> another 6 were hung on the palms trunks at a height of 1.5 m<br />
(aerial traps). The weevils from both traps in the three plantations were collected<br />
weekly, from April to November, <strong>and</strong> transferred to laboratory where their<br />
numbers were recorded. It was found that the monthly average capture of<br />
terrestrial traps was 2–3 folds the aerial traps (Fig. 3).<br />
5.2.3. Density of Traps<br />
A field trial was carried out in UAE to compare the catch of pheromone traps<br />
installed at rates of 1, 2 or 4 traps per ha, in three date palm plantations
220<br />
M.S.T. ABBAS<br />
(Anonymous, 2001). Such plantations contained close total numbers of date<br />
palm trees of the same age, as well as similar levels of infestation. The trial<br />
revealed that the total number of RPW captured within 5 months at the 4 traps<br />
per ha density was 2.4 <strong>and</strong> 2 fold the 1 trap per ha <strong>and</strong> the 2 traps per ha,<br />
respectively. However, the calculated annual costs <strong>and</strong> labor for the 4 traps per<br />
ha was almost 4-fold the 1 trap per ha density. Chinchilla et al. (1993), in<br />
contrast, reported that trap density of 1 per ha was just as effective as 6 traps per<br />
ha, in capturing R. palmarum.<br />
Figure 3. Average monthly numbers of Red Palm Weevils captured <strong>by</strong><br />
terrestrial <strong>and</strong> aerial pheromone traps.<br />
5.2.4. Utilization of Pheromone Traps<br />
Pheromone traps could be utilized for different purposes, including reducing the<br />
population of R. ferrugineus, or estimating the insect population fluctuation <strong>and</strong><br />
its sex ratio in nature.<br />
5.2.4.1. Traps Efficiency<br />
Performance of the pheromone traps could be evaluated <strong>by</strong> estimating<br />
percentages of RPW capture in date palm plantations. An evaluation was carried<br />
out <strong>by</strong> Abbas et al. (2006) in Ras Al-Khaima, UAE during 2000 <strong>and</strong> 2001 <strong>by</strong><br />
releasing marked RPW in three date palm plantations <strong>and</strong> estimating the rate of<br />
capture of the released insects <strong>by</strong> pheromone traps, installed at a density of 1<br />
trap per ha. Adults RPW were marked using small pieces of thin colored plastic,<br />
glued onto the thorax of the insect. Different colors <strong>and</strong> different shapes were<br />
used, representing different date palm plantations (one color per plantation) <strong>and</strong><br />
different dates of release (one shape per release date). Releases were carried out
IPM OF RED PALM WEEVIL<br />
221<br />
at rates of 10–40 individuals per release <strong>and</strong> plantation. During the period from<br />
April to December 2000, only males were released in three date palm<br />
plantations, representing three locations 10–20 km apart from each other (each<br />
plantation contained 12 pheromone traps). Such pheromone traps were inspected<br />
3–4 days post release, <strong>and</strong> the captured weevils were collected <strong>and</strong> transferred to<br />
laboratory where the marked specimens were counted.<br />
During January–December, 2001 both males <strong>and</strong> females of RPW were<br />
marked <strong>and</strong> released in only two plantations (n. 1 <strong>and</strong> 2). In addition, groups of<br />
marked males <strong>and</strong> females were released, periodically, in other four date palm<br />
plantations. Such plantations were among 130 date palm plantations in Ras Al-<br />
Khaima provided with pheromone traps at a rate of 1 trap per ha.<br />
This trapping system was carried out <strong>by</strong> the Ministry of Agriculture in UAE<br />
as a method for controlling RPW. All captured weevils were collected weekly<br />
<strong>and</strong> transferred to the laboratory, thus allowing the monitoring of the released<br />
marked weevils. Percentages of capture <strong>by</strong> pheromone traps did not include<br />
those marked weevils which were captured in the successive weeks after the first<br />
capture (3–4 days post release). Also, they did not include the marked weevils<br />
captured in date palm plantations other than those where they were released. The<br />
study revealed that monthly percentage of marked RPW captured <strong>by</strong> pheromone<br />
traps, 3–4 days post release, from April to December 2000 ranged from 0 to 7%<br />
in plantation 1, from 6 to 27.5% in plantation 2 <strong>and</strong> from 12 to 33% in plantation<br />
3 (Fig. 4). The respective averages in 2001 ranged from 0 to 12.5% in plantation<br />
1 <strong>and</strong> from 3.6 to 31.7% in plantation 2.<br />
Figure 4. Average captures (%) of marked Red Palm Weevils released in three<br />
date palm plantations in 2000 <strong>and</strong> 2001.<br />
The captures of the released weevils did not occur in all releases as no<br />
marked weevils could be captured from 15 releases in plantation 1, 10 releases<br />
in plantation 2 <strong>and</strong> three releases in plantation 3, out of the 32 releases in each<br />
plantation performed during the year 2000. Similarly, no marked weevils could<br />
be captured from 19 releases in plantation 1 <strong>and</strong> 11 releases in plantation 2, out<br />
of 41 releases in 2001. However, the rate of capture reached 80% when 16
222<br />
M.S.T. ABBAS<br />
marked weevils were captured out of 20 released in plantation 2 in the last week<br />
of December, 2000. The percentage of capture of marked females did not differ<br />
significantly from that of marked males in the six plantations in 2001. Averages<br />
of 12.2% of marked males were captured compared to 11.9% marked females.<br />
This study showed that pheromone traps capture both sexes of RPW almost<br />
equally.<br />
The low capture rate in plantation 1 could be attributed to the high rate of<br />
infestation <strong>by</strong> RPW as well as the high incidence of weeds in this plantation.<br />
The high rate of infestation <strong>by</strong> RPW led to the production of high rate of natural<br />
aggregation pheromone (secreted <strong>by</strong> males) <strong>and</strong> kairomones (volatilized from<br />
infested palms), which were much more attractive to released males than<br />
synthetic pheromone <strong>and</strong> kairomone. Kalshoven (1981) reported that volatiles<br />
from infested palms <strong>and</strong> from fermenting palm sap (as a result of infestation)<br />
were well known to attract palm weevils. The high incidence of weeds, in turn,<br />
attracted the weevils as a habitat providing shade <strong>and</strong> shelter. In contrast, the<br />
high rate of capture in plantation 3 could be attributed to the very low rate of<br />
infestation <strong>by</strong> RPW, as well as to the old age of the palm trees (more than 20<br />
years old) in this plantation. Thus, the pheromone <strong>and</strong> kairomone in the traps<br />
were more attractive to the released marked weevils.<br />
5.2.4.2. Estimating RPW Population Fluctuations<br />
Population fluctuation of R. ferrugineus was studied using pheromone traps at a<br />
rate of one trap per ha, to assess the variations in numbers of resident weevils<br />
from 1 plantation to another, to provide epidemiological data about the<br />
infestation levels. Also the study determined the peak(s) of RPW populations<br />
which can help in identifying the best timing of application of protective<br />
chemicals. Abbas et al. (2006) studied the population fluctuation of R.<br />
ferrugineus in three date palm plantations (1, 2 <strong>and</strong> 3) in Ras Al-Khaima, UAE<br />
during 2000 <strong>and</strong> 2001, using the terrestrial pheromone traps. The study revealed<br />
that the populations of the weevils increased gradually to reach a peak in March<br />
or April, <strong>and</strong> then gradually decreased til the end of the year.<br />
The study showed also that the RPW population was much less prevalent in<br />
plantation 3 compared to plantations 1 <strong>and</strong> 2 (Fig. 5). The results showed that<br />
protective chemical insecticidal sprays against RPW in this province should be<br />
started in March, followed <strong>by</strong> a further spray in April.<br />
5.2.4.3. Estimating Reduction of RPW Populations<br />
Continuous use of pheromone traps, changing the pheromone pack <strong>and</strong> the food<br />
substrate (dates or palm tissues) in the proper time, should result in a progressive<br />
decrease of the R. ferrugineus population in the treated areas. The total numbers<br />
of weevils captured <strong>by</strong> pheromone traps in the above mentioned three<br />
plantations (1, 2 <strong>and</strong> 3), for example, were much lower in 2001 compared to<br />
2000. A total of 65,000 weevils were captured within 18 months <strong>by</strong> pheromone
IPM OF RED PALM WEEVIL<br />
223<br />
traps installed in more than 130 date palm plantations in Ras Al-Khaima, site of<br />
the three tested plantations. In agreement with such observations, Oehlschlager<br />
et al. (1993) reported that mass trapping with aggregation pheromone traps<br />
reduced R. palmarum populations <strong>and</strong> the incidence of the associated red ring<br />
disease in oil palm plantations. As for R. ferrugineus, Oehlschlager (2007)<br />
mentioned that there was a strong evidence that trapping, in combination with<br />
chemical spraying, decreased infestation <strong>by</strong> 64%, while smaller scale<br />
experiments indicated that trapping alone reduced infestation <strong>by</strong> 71%.<br />
Muralidharan, Vaghasia, <strong>and</strong> Sodagar (1999) obtained similar results <strong>and</strong><br />
reported that trapping reduced the capture rate of R. ferrugineus <strong>by</strong> 75%, within<br />
3 years.<br />
Figure 5. Population fluctuations of Red Palm Weevilsl in three date palm<br />
plantations in the years 2000 (a) <strong>and</strong> 2001 (b).<br />
5.2.4.4. Estimating Sex Ratios<br />
In field trials no significant differences were observed between response patterns<br />
of female <strong>and</strong> male R. ferrugineus or R. vulneratus to the aggregation<br />
pheromone (Hallett et al., 1993). In agreement with this report, Abbas et al.<br />
(2006) found that when marked RPW males <strong>and</strong> females were released in date<br />
palm plantations the frequencies of captured females did not differ significantly
224<br />
M.S.T. ABBAS<br />
from that of males. Abraham, Faleiro, Shuaibi, <strong>and</strong> Alabdan (2001), however,<br />
reported that R. ferrugineus captured <strong>by</strong> pheromone traps were most likely<br />
female dominated, as the sex ratio in captured weevils was 1 male:2.7 females.<br />
El-Garhy (1996) found this ratio to be 1 male:2 females (in Ismaelyia,<br />
Egypt) while Abbas et al. (2006) found that out of 18,047 RPW captured from<br />
five date palm plantations (Ras Al-Khaima, UAE) during 2000 <strong>and</strong> 2001, the<br />
females represented 60.2% of the total catch, while males represented 39.8%<br />
(almost 1 male:1.51 females). Finally, Abd-Allah <strong>and</strong> Al-Khatri (2005) compared<br />
the catch of different colours of pheromone traps hung on the palm trees at 1 m<br />
height in Sultanate of Oman. These authors found that the orange or red traps<br />
captured almost 2-fold RPW compared to the blue ones. However, sex ratio in<br />
the captured weevils was almost 1 male:1.1 females, in the 3 traps.<br />
5.3. Entomopathogenic Nematodes<br />
EPN from the families Steinernematidae <strong>and</strong> Heterorhabditidae are widely<br />
regarded as being excellent biological control agents for a number of insect pests<br />
in soil <strong>and</strong> cryptic habitats (Gaugler & Kaya, 1990; Kaya & Gaugler, 1993).<br />
They possess many positive attributes including their wide range hosts, safety to<br />
vertebrates, plants as well as non target <strong>org</strong>anisms, exemption from registration<br />
in many countries, ease of in vitro production <strong>and</strong> application using st<strong>and</strong>ard<br />
spray equipments. The two families bear mutualistic bacteria in the intestine,<br />
belonging to the genera Xenorhabdus (in Steinernematidae) <strong>and</strong> Photorhabdus<br />
(in Heterorhabditidae).<br />
The free-living, non-feeding 3rd instars (infective juveniles) of these<br />
nematodes possess attributes of both insect parasitoids or predators <strong>and</strong><br />
entomopathogens. Like parasitoids <strong>and</strong> predators, they have chemo-receptors<br />
<strong>and</strong> are motile; like pathogens, they are highly virulent, killing their host victims<br />
within 24–48 h.<br />
5.3.1. Pathogenicity to RPW<br />
Several laboratory studies were carried out to evaluate the efficiency of EPNs<br />
against larvae <strong>and</strong> adults of R. ferrugineus. Abbas <strong>and</strong> Hanounik (1999) tested<br />
the virulence of Steinernema riobravis, S. carpocapsae (All strain) <strong>and</strong><br />
Heterorhabditis sp. (Egyptian isolate) against larvae <strong>and</strong> adults of RPW. They<br />
found that the three nematode species caused 10–100% mortality in the larvae,<br />
at concentrations ranging from 30 to 240 infective juveniles (IJs) per larva. The<br />
trial was carried out in Petri-dishes lined with filter paper. The LC 50 values were<br />
51, 61 <strong>and</strong> 56.6 IJs per larva for S. riobravis, S. carpocapsae <strong>and</strong><br />
Heterorhabditis sp., respectively. Adults RPW were less susceptible to the<br />
nematode infection, as the corresponding LC 50 values for the three species were<br />
900, 1,100 <strong>and</strong> 1,416 IJs per adult. However, such infected adults produced<br />
2,000–242,000 IJs per weevil, but no correlation was found between dose <strong>and</strong><br />
IJs production.
IPM OF RED PALM WEEVIL<br />
225<br />
Abbas et al. (2001b, 2001c) were able to isolate S. abbasi <strong>and</strong> H. indicus<br />
from RPW adults collected from date palm plantations at Al-Hamranyia, UAE.<br />
They tested the pathogenicity of these two species to larvae <strong>and</strong> adults in Petri<br />
dishes <strong>and</strong> found that 5th larval instar was less susceptible than the 3rd instar to<br />
both species, at concentrations of 100 <strong>and</strong> 200 IJs per larva. The LC 50 values for<br />
3rd <strong>and</strong> 5th instars were 69.2 <strong>and</strong> 97.7 IJs per larva, respectively, for S. abbasi<br />
while for H. indicus they were 123 <strong>and</strong> 128.8 IJs per larva. However, only 11.5<br />
<strong>and</strong> 8.6% of dead RPW larvae infected with S. abbasi <strong>and</strong> H. indicus,<br />
respectively, produced IJs. The average number of IJs produced per larva was<br />
33,000 (2,000–113,000) for S. abbasi <strong>and</strong> 35,000 (5,000–85,000) for H. indicus.<br />
Slight differences in virulence towards adult weevils were found between S.<br />
abbasi <strong>and</strong> H. indicus, at concentrations of 12.5 <strong>and</strong> 25 IJs/cm 2 of s<strong>and</strong> surface,<br />
in a trial carried out in plastic cups lined with moistened sterilized s<strong>and</strong>. No<br />
difference was noticed at concentrations of 50 <strong>and</strong> 100 IJs/cm 2 . The calculated<br />
LC 50 values were 23.2 <strong>and</strong> 25.1 IJs/cm 2 of s<strong>and</strong> for S. abbasi <strong>and</strong> H. indicus,<br />
respectively. Of the dead adults infected with S. abbasi <strong>and</strong> H. indicus, 93 <strong>and</strong><br />
89%, respectively, produced IJs with respective averages of 983,000 (93,000–<br />
3,055,000) <strong>and</strong> 776,000 (145,000–2,820,000) IJs per weevil at the applied<br />
concentration of 100 IJs/cm 2 of s<strong>and</strong>. It should be noted that the recommended<br />
commercial application of EPNs as biocontrol agents was reported to be 2.5– 5⋅<br />
10 9 IJs/ha (Ge<strong>org</strong>is & Hague, 1991). This rate is equivalent to 25–50 IJs/cm 2 of<br />
soil surface.<br />
Saleh <strong>and</strong> Alheji (2003) compared virulence of four species of EPN to the<br />
3rd <strong>and</strong> 8th larval instars, as well as adults of RPW in laboratory. Such tested<br />
nematodes were H. indicus (from Saudi Arabia), H. bacteriophora HP88 (from<br />
USA), S. abbasi (from Sultanate of Oman) <strong>and</strong> S. carpocapsae (from Germany).<br />
A concentration of 100 IJs per larva (in 9 cm Petri dishes lined with filter paper)<br />
was used for the assay with larvae, whereas concentrations of 10–100 IJs/cm 2 of<br />
s<strong>and</strong> surface were used for adults (in 9 cm Petri-dishes lined with 50 g fine<br />
s<strong>and</strong>). The results indicated that 3rd instar larvae were highly susceptible as all<br />
tested nematode species caused 100% mortality within 2–3 days. The 8th instar<br />
larvae were found to be less susceptible, as percentages of mortality were 60%<br />
<strong>by</strong> S. abbasi, 70% <strong>by</strong> H. indicus <strong>and</strong> H. bacteriophora, <strong>and</strong> 80% <strong>by</strong> S.<br />
carpocapsae. RPW adults were also less susceptible to nematode infection than<br />
larvae. Mortality at the tested concentrations, 10–100 IJs/cm 2 of s<strong>and</strong> surface,<br />
ranged from 17 to 75% for H. indicus, from 25 to 83% for H. bacteriophora,<br />
from 33 to 75% for S. abbasi <strong>and</strong> from 33 to 92% <strong>by</strong> S. carpocapsae. The<br />
respective LC 50 values were 49.9, 40.2, 32.4 <strong>and</strong> 6.4 IJs/cm 2 of s<strong>and</strong>. Such LC 50<br />
values correspond to 3,172, 2,555, 2,060 <strong>and</strong> 406 IJs per adult RPW,<br />
respectively.<br />
Shamseldean (2002), however, reported that adult R. ferrugineus was the<br />
most susceptible stage to nematode infection when testing the efficiency of 13<br />
species <strong>and</strong>/or isolates of the Heterorhabditis <strong>and</strong> 2 isolates of Steinernema<br />
against larvae, pupae <strong>and</strong> adults. He stated also that the last instar larva was less<br />
susceptible than the pupa. Shamseldean <strong>and</strong> Atwa (2004) reported that three<br />
Egyptian isolates of Steinernema were highly pathogenic to RPW larvae <strong>and</strong><br />
adults. High mortality rates (100%) were recorded when adults were treated with
226<br />
M.S.T. ABBAS<br />
those 3 isolates, while mortalities in last larval instar ranged between 78 <strong>and</strong><br />
90%.<br />
5.3.2. Field trials<br />
5.3.2.1. Injection of Nematodes<br />
Nematodes injection is carried out <strong>by</strong> making 3–4 artificial tunnels (15–20 cm<br />
deep) using an electrical hammer drill with a 20–40 cm long screw, above <strong>and</strong><br />
around the infested spot, in the palm trunk , where creamy to dark brown sap is<br />
noticed (a symptom of RPW infestation). Nematode suspensions are injected in<br />
such tunnels through perforated plastic tubes inserted into such tunnels. After<br />
injection, the opening of the tunnels are covered with damp soil to avoid<br />
reinfestation.<br />
Shamseldean (2002) carried out field applications of EPN against RPW<br />
infestation (during 1998–2001) <strong>by</strong> injecting the trees with 120 ml of the<br />
nematode suspension at a concentration of 3,000 IJs/ml, injected in each<br />
artificial tunnel with a total of 1,440,000 IJs per tree. The treated date palms<br />
were checked 1 month later <strong>and</strong> during the following 5 months to check the recovery<br />
from infestation. The numbers of treated palms were 36 (in 1998), 45 (in 1999), 30<br />
(in 2000), 27 (in 2001). Egyptian isolates of EPN were used: H. bacteriophora<br />
(strain EKB20), H. indicus (strain EGBB) <strong>and</strong> Steinernema sp. (strain EBNUE).<br />
The author mentioned that the treated palm trees, in all applications, were found<br />
healthy with no symptoms of old or new infestation. Shamseldean <strong>and</strong> Atwa<br />
(2004) stated that injection of three Egyptian isolates of Steinernema in infested<br />
date palm trees resulted in 88.9 <strong>and</strong> 91.9% recoveries when the isolate EGG4<br />
was used, compared to 77.7 <strong>and</strong> 77.1% when the isolate EBNE was used during<br />
2001 <strong>and</strong> 2002, respectively. In 2003, percentages of recoveries obtained were<br />
83.3 <strong>and</strong> 72.2%, <strong>by</strong> EGG4 <strong>and</strong> EIKE isolates, respectively.<br />
Abbas, Saleh, <strong>and</strong> Okil (2001a) applied the same technique of nematodes<br />
injection to seven infested date palm trees, but used another method to evaluate<br />
the efficiency of the injected nematodes. Two weeks after injection the leafaxils<br />
in the treated area was removed until reaching the open of the natural<br />
tunnel made <strong>by</strong> the insect larva. It was interesting that no dead larvae could be<br />
obtained in the treated trees <strong>and</strong> all larvae found were alive <strong>and</strong> healthy. The<br />
nematodes used in this trial were S. abbasi, S. riobravis, S. feltiae, S.<br />
carpocapsae <strong>and</strong> H. bacteriophora. El-Bishry, El-Sebaey, <strong>and</strong> Al-Elimi (2000)<br />
obtained almost similar results.<br />
Another method of injecting nematodes in the infested palm trees was tested<br />
<strong>by</strong> Abbas, Hanounik, Mousa, <strong>and</strong> Al-Bagham (2000). The leaf-axils were<br />
removed from the infested spot on the trunk (showing symptoms of infestation)<br />
until reaching the entrance of the larval tunnel. The tunnels were then injected<br />
with the nematode suspension containing 5,000 IJs/ml after which the entrances<br />
were plugged with damp soil. The area where the leaf-axils were removed was
IPM OF RED PALM WEEVIL<br />
227<br />
also covered with a thick layer of damp soil, to prevent new infestations. Thirty<br />
one tunnels in 25 trees were injected, each with 50–100 ml. of the S. riobravis<br />
suspension. Two weeks later, the injected tunnels were checked for dead <strong>and</strong>/or<br />
alive larvae. Out of the 31 injected tunnels, only four contained nematodeinfected<br />
dead larvae, while 12 tunnels contained alive healthy larvae, with a total<br />
25% mortality. However, no dead or alive larvae could be found in the other 15<br />
tunnels. The absence of larvae in the latter tunnels was interpreted as the larvae<br />
probably migrated through sub-tunnels inside the trunk, before or after the<br />
nematode injection.<br />
Saleh <strong>and</strong> Alheji (2003) used a third method for injecting a nematode<br />
suspension in the infested date palm trees, treating 30 active tunnels, in 20 trees,<br />
with fresh exudates <strong>and</strong> frass, <strong>by</strong> making few small holes with an electric drill at<br />
the site of infestation, to reach the tunnel network in the trunk. A suspension of<br />
H. indicus at the rate of 10,000 IJs/ml was injected through the holes at the site<br />
of infestation, then blocking the holes with soil. Two weeks later, the tunnels<br />
were inspected <strong>and</strong> numbers of dead <strong>and</strong> alive larvae or adults were recorded.<br />
The results indicated that percentages of mortality were 58.8% in larvae <strong>and</strong><br />
43.5% in adults.<br />
In conclusion, the recovery of treated palm trees expressed <strong>by</strong> “no symptoms<br />
of old or new infestation” as mentioned <strong>by</strong> Shamseldean (2002) <strong>and</strong><br />
Shamseldean <strong>and</strong> Atwa (2004) appears controversial. Injecting nematodes in<br />
artificial tunnels around the spot of infestation does not warrant that the infective<br />
juveniles reach RPW larvae inside their tunnels. The walls of the artificial<br />
tunnels form barriers as the IJs can not penetrate such walls <strong>and</strong>/or move<br />
through wood tissues.<br />
El-Bishry et al. (2000) attributed the poor results of injecting nematodes to<br />
the deleterious effect of frass in larval tunnels on the injected IJs. These authors<br />
mentioned that juveniles of five species of EPN were killed within 24 h when<br />
placed on the frass of infested <strong>and</strong> decomposed tissues of date palm. However,<br />
our studies (unpublished) revealed that the feces of RPW larvae <strong>and</strong> frass<br />
obtained from larval tunnels did not affect viability or pathogenicity of infective<br />
juveniles of S. riobravis or H. indicus when placed on such material for 15 days.<br />
The findings of El-Bishry et al. (2000) could be related to the fact that the frass<br />
<strong>and</strong> decomposed tissues of infested palm are subjected to fermentation <strong>by</strong><br />
micro<strong>org</strong>anisms which produce alcohols <strong>and</strong> other toxic materials toxic to the<br />
juveniles.<br />
Compared to nematode injection, the chemical insecticides injected in<br />
artificial tunnels can penetrate such tunnels, are absorbed <strong>by</strong> the wood tissues<br />
<strong>and</strong> may reach the larvae inside their tunnels.<br />
5.3.2.2. Spraying Nematodes<br />
Trunk Spraying<br />
A semi-field trial was conducted <strong>by</strong> Abbas et al. (2000) to estimate the<br />
efficiency of nematodes sprayed against adults of RPW. Sixteen young trees (3–5<br />
years old) were individually caged <strong>by</strong> 2 × 2 × 2 m cages made of wooden frame
228<br />
M.S.T. ABBAS<br />
<strong>and</strong> wire screen. The trunks of 12 trees representing three treatments were<br />
sprayed with one l of nematode suspension containing 2 × 10 6 IJs per tree. The<br />
amount of suspension was enough to wet the whole short trunk <strong>and</strong> was sprayed<br />
carefully so that it did not reach the soil. Two commercial antidesiccants, Liqua-<br />
Gel (Miller Chemicals <strong>and</strong> Fertilizer Corporation, USA) at a rate of 100 ml/l <strong>and</strong><br />
Leaf-Shield (Aquatrols Corporation of America) at a rate of 2.5 g/l, were added<br />
to the nematode suspension in the first <strong>and</strong> second treatments, respectively. The<br />
last four trees were sprayed with water as control. Ten females <strong>and</strong> five males of<br />
RPW were released in each cage immediately after treatment.<br />
The palm trees were inspected daily for 10 days <strong>and</strong> the dead weevils were<br />
transferred to laboratory <strong>and</strong> kept individually in White-traps for extracting the<br />
infective juveniles (IJs) produced <strong>by</strong> the infected insects. Dead weevils which<br />
did not give rise to infective juveniles were dissected to check infection. The<br />
results indicated that mortality in RPW adults was 8.9% when the anti-desiccant<br />
Leaf-Shield was used with nematode suspension <strong>and</strong> 13.3% when Liqua-Gel<br />
was used. However, nematode suspension without anti-desiccant gave 11.7%<br />
mortality.<br />
In general anti-desiccants are utilized with the commercial formulations of<br />
EPN to enhance their persistence <strong>and</strong> performance in the field (Ge<strong>org</strong>is, 1990;<br />
Kaya & Gaugler, 1993). The poor efficacy of S. riobravis sprayed on palm trees<br />
despite the addition of anti-desiccants could be attributed to the adverse effect of<br />
sun heat <strong>and</strong> UV radiation on the IJs. The leaf-axils of palm trees do not provide<br />
enough shade or shelter to IJs. In addition, soil, not leaf-axils, is the natural<br />
habitat for the nematodes.<br />
Hanounik et al. (2000a) carried out a similar trial using a Heterorhabditis sp.<br />
isolated from Saudi Arabia, alone or with Leaf-Shield (100 ml/l of water) or<br />
Liqua-Gel (2.5 g/l of water). The caged date palm trees were first artificially<br />
infested <strong>by</strong> releasing 10 RPW adults on the trunk of each tree <strong>and</strong> 1 h later the<br />
trees were sprayed <strong>by</strong> the nematode suspension. Each tree received an average<br />
of 3.75 × 10 6 IJs in 2 l of water. The trees were inspected daily starting from the<br />
3rd day until the 7th day post-treatment to record weevil mortality. The results<br />
showed that mortalities in R. ferrugineus adults were 65% (<strong>by</strong> using the<br />
nematode alone or with Liqua-Gel) <strong>and</strong> 87.5% (<strong>by</strong> using the nematode with Leaf<br />
Shield). Such results, differ from those obtained <strong>by</strong> Abbas et al. (2000) <strong>and</strong> may<br />
depend on the experimental procedure applied. The RPW adults in procedure of<br />
Hanounik et al. (2000a) were released on the trunks of the palm trees before<br />
spraying the EPN suspension, which means that the weevils were sprayed<br />
directly with the infective nematodes.<br />
5.4. Soil Treatments<br />
According to field studies <strong>and</strong> observations (Abbas et al., 2000), it was<br />
concluded that RPW adults sometimes inhabit soil, probably seeking shade <strong>and</strong><br />
shelter. This conclusion was based on the following reasons: (i) up to 20–100%<br />
of RPW adults collected monthly <strong>by</strong> pheromone traps were found to be
IPM OF RED PALM WEEVIL<br />
229<br />
parasitized with unidentified non pathogenic nematodes, (ii) both S. abbasi <strong>and</strong><br />
H. indicus were isolated from RPW adults (Abbas et al., 2001b, 2001c), (iii)<br />
young date palm trees (3–10 years old) were found to undergo severe infestation<br />
<strong>by</strong> RPW at or below soil surface, (iv) terrestrial pheromone traps were found to<br />
capture 2–3 fold RPW, compared to aerial traps (hung at 1–1.5 m height).<br />
Abraham, Shuabi, Faleira, Abuzuhairah, <strong>and</strong> Vidyasagar (1998) mentioned that<br />
on young growing date palms, the weevils take shelter under the splitting bark<br />
<strong>and</strong> lay eggs within the newly emerging roots.<br />
Ferry <strong>and</strong> Gomez (2002) reported that larvae of R. ferrugineus could be<br />
found in any place within the palm even in the very base of the trunk where the<br />
roots emerge. The emerged adults in this case emerge in the soil. Also, El-<br />
Sebaey (2004a) found that many infested trunk bases of date palm harbored<br />
reliable numbers of RPW surviving in these parts, just under the ground level.<br />
Such weevils were found alive after removing the infested collapsed palms for a<br />
long time <strong>and</strong> infested the growing roots in the soil.<br />
Table 2. Mortality (%) of Rhynchophorus ferrugineus adults released in cages<br />
with soil treated with Steinernema riobravis at a rate of 8 × 10 6 IJs per cage.<br />
Mortality<br />
Treated cages<br />
Untreated<br />
cages<br />
7 8<br />
1<br />
2<br />
3<br />
4<br />
5<br />
6<br />
Total<br />
86.7<br />
46.7<br />
80.0<br />
86.7<br />
73.0<br />
100<br />
20.0<br />
13.8<br />
Due to<br />
nematode<br />
infection<br />
86.7<br />
33.3<br />
60.0<br />
66.7<br />
60.0<br />
86.7<br />
–<br />
–<br />
5.5. Semi-Field Trials<br />
As reported <strong>by</strong> Abbas et al. (2000), eight 3–5 years old date palm trees were<br />
caged individually <strong>by</strong> 2 × 2 × 2 m cages made of wooden frame <strong>and</strong> wire screen.<br />
In six cages, the soil was sprayed with 10 l of EPN suspension with 8 × 10 6 IJs<br />
of S. riobravis, while in the other 2 cages the soil was sprayed with 10 l of<br />
water as control. Ten females <strong>and</strong> five males of RPW were released in each cage<br />
3 h post treatment. The cages were inspected daily <strong>and</strong> the dead weevils were<br />
transferred to laboratory <strong>and</strong> kept in White-traps to extract the IJs produced <strong>by</strong><br />
infected weevils. Dead weevils not giving rise to IJs were dissected to check<br />
infection. The results of this trial (Table 2) showed that S. riobravis caused<br />
considerable mortalities among RPW adults in the treated cages. Average<br />
mortality due to nematode infection was 65.6% (range 33.3–86.7%).<br />
Interestingly, 40% of the dead weevils were found on the trunk at leaf-axils.<br />
Saleh <strong>and</strong> Alheji (2003) conducted similar trial <strong>by</strong> using S. carpocapsae <strong>and</strong><br />
H. bacteriophora at a rate of 2 million IJs in 3 l of water per tree. The trial was<br />
carried out in Saudi Arabia in February, with daily mean temperature between 8<br />
<strong>and</strong> 20°C. Steinernema carpocapsae caused 77.5% mortality in RPW adults
230<br />
M.S.T. ABBAS<br />
while H. bacteriophora caused only 17.5 % mortality. The authors mentioned<br />
that the low effect of H. bacteriophora could be interpreted as this species was<br />
isolated from a tropical area, therefore it was not adapted to low prevailing<br />
temperatures. Such findings confirm the importance of the biological <strong>and</strong><br />
ecological characteristics of the EPN applied, since soil is the natural habitat of<br />
EPN <strong>and</strong> most of the successful control with EPNs was achieved against soilinhabiting<br />
insects (Ge<strong>org</strong>is, 1990).<br />
In conclusion, soil application of EPNs could be recommended as a<br />
biological tool for RPW control, within a durable IPM strategy. Persistance after<br />
release is a fundamental property of any biocontrol agent, in view of its practical<br />
exploitation. Steinernema abbasi <strong>and</strong> H. indicus, sprayed in a field study around date<br />
palms, survived in the treated soil for at least 1 year (Abbas & Mousa, 2003).<br />
REFERENCES<br />
Abbas, M. S. T., & Hanounik, S. B. (1999). Pathogenicity of entomopathogenic nematodes to red<br />
palm weevil, Rhynchophorus ferrugineus. International Journal of Nematology, 9, 84–86.<br />
Abbas, M. S. T., Hanounik, S. B., Mousa, S. A., & Al-Bagham, S. H. (2000). Soil application of<br />
entomopathogenic nematodes as a new approach for controlling Rhynchophorus ferrugineus on<br />
date palm. International Journal of Nematology, 10, 215–218.<br />
Abbas, M. S. T., Hanounik, S. B., Mousa, S. A., & Awash, S. A. (2001b). Isolation of<br />
entomopathogenic nematodes from Ras Al-Khaima <strong>and</strong> Al-Fugaira Emirates (UAE). Egyptian<br />
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Gopinadhan, P. B., Moh<strong>and</strong>as, N., & Nair, K. P. V. (1990). Cytoplasmic polyhedrosis virus infecting<br />
red palm weevil. Current Science, 59, 577–580.<br />
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Gunawardena, N. E., & B<strong>and</strong>arage, U. K. (1995). 4-Methyl-5-Nonanol (Ferrugineol) as an<br />
aggregation pheromone of the coconut pest, Rhyncophorus ferrugineus. Journal of the National<br />
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Hallett, R. H., Oehlschlager, A. C., Gries, G., Angerilli, N. P. D., Alshareqi, R. K., Gassouma, M. S.,<br />
et al. (1993). Field testing of aggregation pheromone of two Asian palm weevils. International<br />
Palm Oil Congress, 20–25 September, 1993, Kualalumpur, Malysia.<br />
Hamdi, A. N. (1998). Report on present status of Red Palm Weevil <strong>and</strong> Date Palm borers in Bahrain.<br />
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Rhynchophorus ferrugineus on date palm trees. International Journal of Nematology, 10, 131–134.<br />
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Biological control of Rhynchophorus ferrugineus as a major component of IPM (pp. 125–150).<br />
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38, 181–206.<br />
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weevil, Rhynchophorus ferrugineus. Phytoparasitica, 27, 107–108.<br />
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10<br />
CONTROL OF URTICATING LEPIDOPTERA<br />
OUTBREAKS WITH BACILLUS THURINGIENSIS<br />
AERIAL TREATMENTS<br />
PIO FEDERICO ROVERSI, LEONARDO MARIANELLI,<br />
LORENZO MARZIALI, MICHELE SQUARCINI AND<br />
GIANPAOLO BARZANTI<br />
Agricultural Research Council,<br />
Research Centre for Agrobiology <strong>and</strong> Pedology,<br />
Cascine del Riccio,<br />
50125 Firenze, <strong>Italy</strong><br />
Abstract. The main species of urticating Lepidoptera are presented, together with the environmentfriendly<br />
methods based on biological control agents. These include the bacterium Bacillus thuringiensis<br />
<strong>and</strong> the technologies developed to treat large park <strong>and</strong> forest areas, in wild as well as urban environments.<br />
Advances in the aerial control methods developed <strong>and</strong> the effects of formulations on the treatments<br />
efficacy <strong>and</strong> persistence are briefly described.<br />
1. INTRODUCTION<br />
A limited number of Lepidoptera is considered as seriously harmful in forest <strong>and</strong><br />
urban parks <strong>and</strong> this characteristic is linked to the possibility that massive population<br />
explosions may occur (Myers, 1988). From the ecological point of view, dramatic<br />
density changes or “outbreaks” are phenomena common to various animal species,<br />
including insects, <strong>and</strong> occur through cycles of increasing population density changes<br />
(Berryman, 1987). The capability to increase enormously in number <strong>and</strong> to attack<br />
trees in normal-growing conditions, acting as a prime debilitating or “early damagecausing<br />
biotic factor” makes the infestation of some species of defoliating<br />
Lepidoptera particularly dangerous. Furthermore, their attacks can predispose trees<br />
to infections <strong>by</strong> pathogenic agents, that exploit the reduced capability of the host to<br />
react.<br />
Among Lepidoptera there are species noted not only for the direct damage<br />
caused <strong>by</strong> defoliating activities, but also for their capability to interact with agro-<br />
235<br />
A. <strong>Ciancio</strong>, K.G. Mukerji (eds.), Integrated Management of Arthropod Pests<br />
<strong>and</strong> Insect Borne Diseases, Integrated Management of Plant Pests <strong>and</strong> Diseases 5,<br />
DOI 10.1007/978-90-481-8606-8_10, © Springer Science+Business Media B.V. 2010
236<br />
P.F. ROVERSI ET AL.<br />
forestry productions <strong>and</strong> other human activities, including aspects related to<br />
environmental hygiene. To this instance are referred those species whose larvae,<br />
during specific developmental stages, bear urticating hairs, i.e. tegumentary<br />
appendages, connected to special gl<strong>and</strong>s, capable of eliciting adverse reactions in<br />
humans rangin from dermatitis <strong>and</strong> conjunctivitis to Ig-E mediated anaphylactic<br />
reactions (Wirtz, 1984; Arlian, 2002).<br />
In this chapter recent advance on these issues are discussed, with particular<br />
attention to environment-friendly methods based on biological control agents,<br />
including the G+ bacterium Bacillus thuringiensis <strong>and</strong> the technologies developed to<br />
treat large park <strong>and</strong> forest areas in wild as well as urban environments.<br />
2. URTICATING LEPIDOPTERA<br />
The larval hairs, which act as defence mechanisms, are very small (about one tenth<br />
of mm) <strong>and</strong> are generally harpoon-shaped. Their dissemination in the environment<br />
raises serious implications for the public hygiene. When hairs penetrate the skin <strong>and</strong><br />
mucosal tissues of man or other warm-blooded <strong>org</strong>anisms, they cause severe<br />
irritations due to both the physical action of penetration (favoured <strong>by</strong> their shape)<br />
<strong>and</strong> the chemical activity of a soluble protein released <strong>by</strong> the accidental breaking of<br />
the hairs. These structures are set up on the larval body in particular areas called<br />
“mirrors”, whose morphology <strong>and</strong> distribution are characteristic for each species.<br />
The “mirrors” are produced at every moult, reaching their maximum breadth in last-age<br />
larvae that can present from hundred–thous<strong>and</strong> to, sometimes, million urticating<br />
hairs (Fig. 1b, c).<br />
The effects produced on man <strong>by</strong> urticating hairs present a remarkable interest in<br />
health-care, either for epidermic reactions, more or less persistent, aroused on the<br />
majority of victims or for other consequences, sometimes observed in individuals<br />
particularly responsive or sensitized, owing to reiterated contacts. Some worthmentioning<br />
effects are those related to mucous tissues <strong>and</strong> sensory <strong>org</strong>ans, mainly<br />
eyes. Inflammatory reactions can be particularly dangerous for main airways when<br />
massive inhalation occurs, due to unsafe operations performed during pest control<br />
<strong>by</strong> workers not adequately protected (Lamy, Novak, Duboscq, Ducombs, &<br />
Maleville, 1988).<br />
Thanks to their tiny size, urticating hairs are easily carried away <strong>by</strong> air currents.<br />
For this reason, during intense <strong>and</strong> widespread outbreaks, remarkable drawbacks<br />
may occur not only close or within areas stricken <strong>by</strong> the disease, but also in<br />
locations considerably far. In recent years, when monitoring the diffusion of this <strong>and</strong><br />
other structures or arthropods parts, these phenomena were referred as “Animal<br />
Atmospheric Pollution”. At the same time, monitoring operations of pollen <strong>and</strong> other<br />
allergenic structures transported <strong>by</strong> air are performed on this kind of <strong>org</strong>anic<br />
materials (Lamy, 1990; Werno & Lamy, 1990; Gottschling & Meyer, 2006).<br />
Lepidopteran larvae bearing urticating hairs with a defence function are known<br />
among many species of temperate <strong>and</strong> tropical regions within the following families:<br />
Thaumetopoeidae, Lymantriidae, Saturniidae, Nymphalidae, Lasiocampidae,<br />
Bom<strong>by</strong>cidae, Arctiidae, Noctuidae, Anthelidae, Eupterotidae, Limacodidae <strong>and</strong><br />
Megalopygidae.
AERIAL BT TREATMENTS<br />
237<br />
The main species of urticating Lepidoptera, responsible of severe infestations<br />
among countries around the Mediterranean see, belong to the genus Thaumetopoea<br />
(Fam. Thaumetopoeidae) <strong>and</strong> Euproctis (Fam. Lymantridae) (Roversi, 2006). In the<br />
Palaearctic region, the members of the Thaumetopoeidae family form a small group<br />
of species that represents a formidable menace in wide areas even because of the<br />
progressive expansion of their distribution range. The increase in their distribution<br />
area is the consequence of both general climatic trends, characterized <strong>by</strong> milder<br />
winter temperatures, <strong>and</strong> anomalous climatic events allowing colonization of new<br />
territories, either at higher altitudes as well as in areas northern than those reached<br />
until a few years ago.<br />
The two main species known for the negative effects of their infestations are the<br />
Pine Processionary Moth (PPM), Thaumetopoea pityocampa (Den. et Schiff.) <strong>and</strong><br />
the Oak Processionary Moth (OPM), T. processioneae (L.). Proceeding towards<br />
northern territories other species are worth mention, such as T. pinivora (Treitschke)<br />
whose colonies are reported to have increased their extension in areas of North<br />
Europe completely undamaged until recent times.<br />
The individuals of the three species exhibit a sub-social behaviour, their larvae<br />
living in groups throughout their development. Moreover, the first two species<br />
sometimes build nests of remarkable dimensions, so that a huge amount of urticating<br />
hairs can be present inside the nests for a long time.<br />
PPM is a lepidopteran with a wide distribution range in the Mediterranean area<br />
<strong>and</strong> Middle-East Europe. It is considered the most important insect pest of pines in<br />
southern Europe <strong>and</strong> North Africa, affecting many indigenous <strong>and</strong> exotic pines, as<br />
well as other Pinaceae (in order of preference, Pinus nigra austriaca, P. sylvestris,<br />
P. laricio, P. pinea, P. halepensis, P. pinaster, P. canariensis, Cedrus spp. <strong>and</strong> Larix<br />
decidua) (OEPP/EPPO, 2004). Within its range of distribution, T. pityocampa is<br />
common in extremely diversified habitats, varying from coastal formations to<br />
mountain woods at altitudes higher than 2,000 m. Particularly severe problems are<br />
reported at the end of winter, when long processions of mature larvae ab<strong>and</strong>on pines<br />
in a line, as they come down from trees to deepen themselves into the ground, where<br />
pupation will take place (Fig. 1a). In this last phase, contacts with people <strong>and</strong><br />
animals are very frequent.<br />
OPM is an univoltine forest defoliator of deciduous oaks, widely distributed in<br />
central, western <strong>and</strong> southern Europe (Agenjo, 1941). The larvae are equipped, from<br />
the third instar, with urticating hairs <strong>and</strong> are active in spring–summer. They exhibit a<br />
gregarious behaviour throughout their life, constructing sack-shaped nests on the<br />
stem or axis of large branches, in which they pupate in a papery cartoon. This pest<br />
can completely defoliate oak st<strong>and</strong>s but it is also found on isolated trees in avenues<br />
<strong>and</strong> parks. Since the 1990s, heavy attacks <strong>by</strong> OPM have become increasingly<br />
frequent throughout very large areas in various European countries (Flemming,<br />
1997; Tomiczek & Krehan, 2003; Lövgren & Dalsved, 2005; Wulf & Pehl, 2005),<br />
including Holl<strong>and</strong>, where outbreaks had not been reported for a century (Bosma &<br />
Jans, 1998; Stigter & Romeijn, 1992; Stigter, Geraedts, & Spikers, 1996).<br />
In recent years, OPM became a problem even in United Kingdom (Townsend,<br />
2007). In southern Europe heavy <strong>and</strong> extensive infestations occurred both in Middle<br />
European oak environments <strong>and</strong> forests, <strong>and</strong> in sub-Mediterranean inhabited mainly
238<br />
P.F. ROVERSI ET AL.<br />
<strong>by</strong> the Turkey oak Quercus cerris (Camerini, Caronni, & Roversi, 2002; Roversi,<br />
2002). Nest construction on oak stems not only enhances risk of accidental contacts<br />
in green areas but, mostly represents a considerable hazard for forest-workers<br />
committed to carry out coppice cut or to collect firewood.<br />
Figure 1. Thaumetopoea pityocampa larval procession (a), dorsum detail of a<br />
mature larva with a “mirror” of urticating hairs (b, white circle) <strong>and</strong> SEM<br />
magnified densely thickened urticating hairs of a “mirror” (c)<br />
Euproctis chrysorrea (L.), a moth widespread in North Africa <strong>and</strong> Europe<br />
including <strong>Italy</strong>, has been introduced also to North America. This species is common<br />
from the sea level up to the beech mountain altitude, <strong>and</strong> is also frequent in coastal<br />
environments on Arbutus unedo <strong>and</strong> in inl<strong>and</strong> regions on oaks <strong>and</strong> various<br />
Rosaceae shrubs, particularly Crataegus spp. On the latter it forms permanent<br />
hotbeds even in urban <strong>and</strong> suburban parks. During heavy infestations it can defoliate<br />
entire woods, making them unfit to deploy. Since the second instar, Euproctis larvae<br />
bear, on their back, dense str<strong>and</strong>s of tiny urticating hairs, 0.1 mm long, with tricuspidate<br />
tip.<br />
Equally important cases are reported in other geographic areas. A clear example<br />
is the leaf skeletonizer Uraba lugens Walker (Lepidoptera Nolidae), a serious pest of<br />
forestry <strong>and</strong> Eucalyptus st<strong>and</strong>s, particularly in risky areas (e.g., urban zones or near<br />
waterways). Uraba lugens is widespread in the majority of Australian territory<br />
where periodic outbreaks occur which can lead to extensive defoliations. The<br />
species is well established also in new Zeal<strong>and</strong> (Farr, 2002; Mansfield et al., 2006).<br />
The larvae of U. lugens bear, on their back, hairs that after being thrust into man
AERIAL BT TREATMENTS<br />
239<br />
skin inject istamine, causing irritation, sometimes severe, <strong>and</strong> wide itching rash<br />
(Southcott, 1978).<br />
Lepidoptera families including urticating species are present <strong>and</strong> spread in almost<br />
every continent except the most cold regions. Among them the Limantriidae is the most<br />
important one, due to the genus Euproctis. In addition to the two species E. chrysorrhoea<br />
(Fig. 2) <strong>and</strong> E. similis (Fuessly), worth mention are also E. edwardsii (Newman) in<br />
Australia on Eucalyptus spp., E. lunata Walker on Acacia trees in the Indian region,<br />
E. scintillans (Walker) on Robinia pseudoacacia L., E. bipunctapex Hampson in<br />
Singapore <strong>and</strong> E. pseuconspersa (Str<strong>and</strong>) in Japan (Ooi, Goh, Loe, & Goh, 1991; Dunlop<br />
& Freeman, 1997; Ohtaki & Takino, 1998; Balit, Ptolemy, Geary, Russel, & Isbistes,<br />
2001; Subramanian & Krishnamurthy, 2002; Kalia & P<strong>and</strong>ey, 2004).<br />
Figure 2. Euproctis chrysorrhoea: detail of a tuft of urticating hairs with tri-cuspidate tips.<br />
Many authors reported reactions of “tussockosis” to irritating setae of the<br />
Douglas Fir Tussock Moth larvae, Orgyia pesudotugata (McDunnough) in the US<br />
Northwest (Perlman, Press, Googins, Malley, & Poareo, 1976; Press et al., 1977).<br />
Moreover, in some species, adult females rather than larvae exhibit urticating hairs<br />
such as in African <strong>and</strong> South American species belonging to the genus Anaphe<br />
(Family Notodontidae) <strong>and</strong> to the genus Hylesia (Family Saturniidae), like A. p<strong>and</strong>a<br />
(Boisduval), H. urticans Floch & Abonnenc, H. iola Dyar <strong>and</strong> H. lineata (Druce)<br />
(Lamy, Pastureaud, Novak, & Ducombs, 1984). The reactions caused <strong>by</strong> adult moths<br />
or butterflies are called “Lepidopterism”. Damages to people <strong>and</strong> animals are caused<br />
in this case <strong>by</strong> barbed setae in the anal tuft (Fig. 2), the tips of which show gl<strong>and</strong>s<br />
secreting a toxin, normally released <strong>by</strong> female on egg clusters as an effective<br />
deterrent against egg predators <strong>and</strong> parasitoids, like i.e. the Lycenidae Eumaeus<br />
atala florida Rueber (Rotschild, Reichstein, Von Euw, Aplin, & Harman, 1970) <strong>and</strong><br />
the Thaumetopoeidae Ochrogaster lunifer Herrich-Schäffer (Floater, 1998).
240<br />
P.F. ROVERSI ET AL.<br />
3. AERIAL CONTROL<br />
In the last decades, the increasing need to carry out direct monitoring interventions<br />
as a consequence of diffused infestations of urticating species, showed the limit of<br />
control means deployed only after damages was already assessed. It is important to<br />
underline that the use of biocides to reduce large phytophagous populations cannot<br />
solve, in the short term, public health <strong>and</strong> hygiene problems. In fact, the mass of<br />
urticating hairs can remain for a long time in the environment rendering the areas hit<br />
<strong>by</strong> infestations unfit for any use, even for many years.<br />
From this overall picture of serious issues raised <strong>by</strong> lepidopteran infestations<br />
<strong>and</strong> given that, in general, the interventions are set up in forest ecosystems in which<br />
wide range pesticides are not allowed because of their negative environmental<br />
fallout, new adequate strategies must be promoted. Among them, it is necessary to<br />
combine the set up <strong>and</strong> maintaining of efficient monitoring task forces, to forecast<br />
the beginning of new attacks, with the improvement of methods <strong>and</strong> means for the<br />
timely deploy of biopesticides with a low environment impact.<br />
Formulations of B. thuringiensis var. kurstaki (Btk), a naturally sporulating soil<br />
bacteria, have been used for years in North America <strong>and</strong> Europe against lepidopteran<br />
defoliators, in coniferous <strong>and</strong> broad-leaved woods (Martin & Bonneau, 2006; Van<br />
Frankenhuyzen & Payne, 1993; Van Frankenhuyzen, 2000; Roversi, 2008). The<br />
formulations are chosen on account of their effectiveness <strong>and</strong> specificity, as well as<br />
of the rapidity with which the spores are killed <strong>by</strong> the UV radiation (Wilson &<br />
Benoit, 1993; Leong, Cabo, & Kubinski, 1980).<br />
In Canada <strong>and</strong> USA, most of the treatments are applied with airplanes. In <strong>Italy</strong>,<br />
as well in other European countries like France <strong>and</strong> Germany, helicopters are<br />
preferred for control of defoliator lepidopterans, because of their small size <strong>and</strong> the<br />
more or less irregular borders of the areas to be treated. Further reasons are the close<br />
association of the treated surfaces with cultivated areas or the general morphology of<br />
their environments, which rarely present uniform l<strong>and</strong>scapes over large surfaces<br />
(Lentini & Luciano, 1995; Luciano & Lentini, 1999; Martin & Bonneau, 2006).<br />
For aerial spreading of Btk formulations, helicopters have proved more useful<br />
when wind speed is less than 16 kmh, to reduce drift. The best equipment is the<br />
electrically operated rotary nozzle, mounted on bars to wet at ultra-low swath<br />
intervals of about 30 m at each flight. GPS equipments proved also useful to record<br />
both the flight <strong>and</strong> the complete treatment coverage.<br />
Btk spraying experiments carried out in New Zeal<strong>and</strong> against the Tussock Moth<br />
Uraba lugens Walker, proved the reliability of an ULVA-8 spinning disc operating at<br />
12,500 rpm <strong>and</strong> mounted above a track conveyor belt to obtain very small droplets,<br />
with a median volume diameter of 150 μm, varying the dosis applied <strong>by</strong> changing the<br />
belt speed <strong>and</strong> the flow rates (Mansfield et al., 2006). In Spain, Pascual, Robredo, <strong>and</strong><br />
Galante (1990) showed that aerial treatments using a plane distributing soluble<br />
powders of Btk at the dose of 5 l/ha 1 (1,500 cc of commercial product with 8,500<br />
u.i./mg 1 <strong>and</strong> 3.5 l of water), resulted in high mortality of OPM larvae, in colonies<br />
artificially transferred to areas that were then experimentally treated.<br />
Unlike st<strong>and</strong>ard protocols today available for other harmful defoliators of<br />
mesophilous forests, i.e. Lymantria dispar (L.), noxious also to cork oak in North
AERIAL BT TREATMENTS<br />
241<br />
Africa, or Choristoneura fumiferana (Clem.), which is often very dangerous to many<br />
nearctic conifer st<strong>and</strong>s (Lentini & Luciano, 1995; Bauce, Carisey, Dupont, & Van<br />
Frankenhuyzen, 2004), no st<strong>and</strong>ard protocols are available thus far in <strong>Italy</strong> for Btk<br />
products aimed to control main urticating lepidopteran defoliators. Data are now<br />
available only on T. pityocampa, based on experiments proceeding from other<br />
countries. In <strong>Italy</strong>, observations began in the 1960s (De Bellis & Cavalcaselle,<br />
1969; Triggiani & Sidor, 1982; Currado & Brussino, 1985; Niccoli & Tiberi, 1985;<br />
Ambrosi, Salvatori, & Zanotelli, 1993; Battisti, Longo, Tiberi, & Triggiani, 1998).<br />
Further investigations on the capability of aerial treatments <strong>by</strong> means of<br />
biopesticides against PPM were carried out also in other European countries,<br />
especially in France where this species is often noxious mostly in tourist areas, i.e. in<br />
the Maritime Alps (Demolin, Martin, & Lavanceau, 1993; Demolin & Martin, 1998;<br />
Martin & Bonneau, 2006).<br />
Very few data are available for the Brown Tail Moth (BTM) E. chrysorrhoea as<br />
well as for OPM. The latter species, has spread recently northwards in Europe<br />
convincing some EU Member States to introduce national or regional control<br />
programmes for public health reasons (EFSA, 2009). However, only in 2008 an<br />
experimental protocol has been issued <strong>by</strong> means of aerial spreading of Btk over<br />
large areas. Employ doses were stated at 2.5 l/ha 1 of 12.7 BIU (Billion International<br />
Units)/l of commercial formulation <strong>and</strong> were distributed at ultra-low volume at the<br />
time of bud opening, against 1st <strong>and</strong> 2nd instar larvae (Roversi, 2008).<br />
Before aerial Btk treatments are deployed, it is also useful to know the exact<br />
time of presence of larvae, which varies normally according to the different<br />
urticating. For instance, OPM <strong>and</strong> BTM have different larval presence. In <strong>Italy</strong>, for<br />
the former species it is necessary to treat <strong>by</strong> the end of April or at the beginning of<br />
May, when buds are opening <strong>and</strong> leaves growing. However, it is important to treat<br />
larvae before they reach the third instar, when they become urticating. Early<br />
treatments in spring are also capable to better wet the crowns inside. In fact, to reach<br />
a good biopesticide spraying all over the new foliage it is necessary to avoid some<br />
larval groups to escape.<br />
For BTM, the different life cycle patterns lead to treatments in the late summer<br />
or autumn, just before the larvae hide themselves inside winter nests. However, in<br />
mild Mediterranean climates with mild winters where BTM can feed <strong>and</strong> survive on<br />
mixed scrubs, treatments can be delayed to the end of autumn. As to PPM,<br />
treatments can be performed <strong>by</strong> the end of summer, when the newly hatched larvae<br />
start to feed on needles. The winter control of PPM is possible <strong>by</strong> means of Btk<br />
formulations applied on third instar larvae or more (L4–L5) (Martin & Mazet,<br />
2001). Furthermore, it is worth to remark that PPM can show different life cycle<br />
patterns, according to the different seasonal conditions <strong>and</strong> climates. In fact, PPM<br />
eggs can be laid sometimes also at the beginning of autumn (Battisti, 1989).<br />
Numbers of researches have been carried out in the recent years also on the Btk<br />
impact on non-target species, as well as on the persistence of the microbial products<br />
in the treated environment (i.e., spores-crystal complex), or the host plant effects<br />
(Cooke & Régnière, 1999; Appel & Schultz, 1994; Kouassi, Lorenzetti, Guertin,<br />
Cabana, & Mauffette, 2001; Bauce, Bidon, & Berthiaume, 2002; Carisey, Bauce,<br />
Dupont, & Miron, 2004), so that the Btk residual activity is now a key-factor in
242<br />
P.F. ROVERSI ET AL.<br />
operational forestry <strong>and</strong> urban programs (Gindin, Navon, Protasov, Saphis, &<br />
Mendel, 2007).<br />
Figure 3. Petri dish with Btk colonies developing from already died 2nd instar larvae<br />
collected in the field after an aerial treatment.<br />
In experimental assays carried out in spring 2004 on Turkey oak woods in<br />
Tuscany (Central <strong>Italy</strong>), coinciding with the early phase of a new T. processionea<br />
outbreak, a wide aerial Btk treatment was carried out, followed <strong>by</strong> a 1-month<br />
evaluation of its effect on non-target lepidopterans. The control area was checked<br />
daily with traps placed underneath the crowns (Roversi, Rumine, & Barzanti, 2006).<br />
These trials showed a low effect of the treatment against OPM, with a small number<br />
of dead larvae of other species (Roversi et al., 2006).<br />
Figure 4. Numbers of Btk colonies developed from 1 ml water washings of Turkey Oak leaves<br />
collected from the upper part of the tree crowns, after treatment with 31.75 Btk BIU/ha, at<br />
Berignone Forest (Tuscany, Central <strong>Italy</strong>). Leaves were collected in a period of about months<br />
(Bars show st<strong>and</strong>ard deviation) (Roversi et al., unpublished).
AERIAL BT TREATMENTS<br />
243<br />
Further laboratory analyses of both the insects midgut <strong>and</strong> leaves revealed the<br />
presence of bacterial spores inside the whole crown, together with the development<br />
of colonies from 100% of the OPM larval cultures. These were obtained from larvae<br />
died within the first 9 days after the treatment (Fig. 3). Further controls of Btk<br />
persistence using agar cultures of water washings from leaves, collected at both high<br />
<strong>and</strong> medium crown levels, revealed a marked reduction of the living spores 10 days<br />
after the treatments (Fig. 4). In some cases, on the contrary, colonies of Btk spore<br />
were obtained from leaves collected 2 months or more, after treatments (Roversi et<br />
al., unpublished data).<br />
Other field experiments confirmed the persistance of Btk applications based on<br />
milk formulations, used successfully against T. wilkinsonii Tams in Israel. Data<br />
showed that the formulation has a rain-fasting effect, resulting in the retaining of<br />
more than half of the Btk activity after 8 days (Gindin et al., 2007).<br />
In conclusion, the exploitation of biopesticides based on Btk is likely to be<br />
strongly increased in the future, owing to both the scientific evolution <strong>and</strong> the<br />
government policies, encouraging the use of alternative pest control products.<br />
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Martin, J. C., & Bonneau, X. (2006). Bacillus thuringiensis, 30 ans de lutte contre les chenilles<br />
defoliatrices en forêt. Phytoma, 590, 4–7.
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Martin, J. C., & Mazet, R. (2001). Lutte hivernale contre la processionaire du pin. Possibilité d’utilisation<br />
du Bacillus thuringiensis K. Phytoma, 540, 32–35.<br />
Myers, J. H. (1988). Can a general hypothesis explain population cycles of forest lepidoptera? Advances<br />
in Ecological Research, 18, 179–242.<br />
Niccoli, A., & Tiberi, R. (1985). Impiego di Bacillus thuringiensis Berliner nel controllo di insetti dannosi<br />
in ambienti agrari e forestali. Redia, 68, 305–322.<br />
OEPP/EPPO. (2004). Thaumetopoea pityocampa. Bulletin OEPP/EPPO, 34, 295–297.<br />
Ooi, P. L., Goh, K. T., Lee, H. S., & Goh, C. L. (1991). Tussockosis: An outbreak of dermatitis caused <strong>by</strong><br />
tussock moth in Singapore. Contact dermatitis, 24, 197–200.<br />
Ohtaki, N. & Takino, C. (1998). Caterpillar dermatitis in 1977–1996 at Kudanzaka Hospital, Tokio.<br />
Medical Entomology <strong>and</strong> Zoology, 49, 65–68.<br />
Pascual, J. A., Robredo, F., & Galante, E. (1990). Tratamientos aéreos ULV con alfa-cipermetrina,<br />
siflubenzurón y Bacillus thuringiensis contra la procesionaria del roble (Thaumetopoea<br />
processionea) (Lep., Thaumetopoeidae). Boletin Sanidad Vegetal Plagas, 16, 585–591.<br />
Perlman, F., Press, E., Googins, J. A., Malley, A., & Poareo, H., (1976). Tussockosis: Reactions to<br />
Douglas fir moth. Annals of Allergy, 36, 302–307.<br />
Press, E., Perlman, F., Everett, J. R., Googins, J. A., Poareo, H., & Jones, K. (1977). Health hazards to<br />
timber <strong>and</strong> forestry workers from the Douglas fir tussock moth. Archives of Environmental Health,<br />
32, 206–210.<br />
Rotschild, M., Reichstein, T., Euw, J. von, Aplin, R., & Harman, R. R. M. (1970). Toxic Lepidoptera.<br />
Toxicon, 8, 293–299.<br />
Roversi, P. F. (2002). Dinamica di popolazione di Thaumetopoea processionea (L.): Indicatori biologici<br />
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185–192.<br />
Roversi, P. F. (2006). Lepidotteri urticanti. In Allergologia e Dermatologia Entomologiche. Identificazione<br />
dei principali artropodi causa di reazioni locali e sistemiche (pp. 83–91). Accademia nazionale<br />
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Roversi, P. F. (2008). Aerial spraying of Bacillus thuringiensis var. kurstaki for the control of<br />
Thaumetopoea processionea in Turkey Oak Woods. Phytoparasitica, 36, 175–186.<br />
Roversi, P. F., Rumine, P., & Barzanti, G. P. (2006). Efficacia di trattamenti aerei con Bacillus<br />
thuringiensis var. kurstaki per il controllo della processionaria della quercia e impatto sulla<br />
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Southcott, R. V. (1978). Lepidopterism in the Australian region. Records of the Adelaide Children's<br />
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Section 3<br />
MITES BIOLOGICAL CONTROL AND IPM
11<br />
IPM POTENTIALS OF MICROBIAL PATHOGENS<br />
AND DISEASES OF MITES<br />
LEO P. S. VAN DER GEEST<br />
IBED, Section Population Biology<br />
University of Amsterdam,<br />
1098SM<br />
Amsterdam, The Netherl<strong>and</strong>s<br />
Abstract. An overview is given of diseases in mites, caused <strong>by</strong> infectious micro<strong>org</strong>anisms. Many<br />
pathogens play an important role in the regulation of natural populations of mite populations <strong>and</strong> are for<br />
this reason subject of research on the feasibility to develop such pathogens to biological control agents.<br />
Several examples are given of successful application of pathogens for the control of mite pests, but also<br />
failures are discussed. Most studies concern fungal pathogens of tetranychids <strong>and</strong> eriophyids; some of<br />
these fungi are possible c<strong>and</strong>idates for biological control agent of species of noxious mites. An interesting<br />
group of pathogens form the intracellular symbionts: bacteria that may cause unusual effects in their<br />
hosts, such as parthenogenesis, feminization, male killing <strong>and</strong> incompatibilities. This group of bacteria is<br />
present in many invertebrates species <strong>and</strong> are presently widely studied as new molecular techniques have<br />
become available that make detection of such symbionts possible. Attention is also given to quality<br />
control of beneficial mites that are being used in integrated control programs. Beneficial mites, as e.g.<br />
predatory mites, may also be infected <strong>by</strong> micro<strong>org</strong>anisms (bacteria, viruses, microsporidia), resulting in<br />
poor performance of the predator. Prospects for the application of pathogens in IPM systems are<br />
discussed.<br />
1. INTRODUCTION<br />
As other <strong>org</strong>anisms, Acari may also be subject to disease, usually caused <strong>by</strong><br />
pathogenic micro<strong>org</strong>anisms. Our knowledge on pathogens of mites, however, is still<br />
fragmentary, in contrast to what we know about pathogens of insects. The rapid<br />
development of invertebrate pathology in the second half of the twentieth century<br />
has largely been due to the study of insect pathogens. Relatively few mite pathogens<br />
are known, despite the large number of mite species. Approximately 48,000 species<br />
have hitherto been described <strong>and</strong> it is estimated that this number represents only<br />
10% of the total number of mite species.<br />
That mite pathogens have been studied less comprehensively is not surprising:<br />
their frequently small size renders disease diagnosis often difficult <strong>and</strong><br />
pathophysiogical studies almost impossible. From the other h<strong>and</strong>, the often large<br />
249<br />
A. <strong>Ciancio</strong>, K.G. Mukerji (eds.), Integrated Management of Arthropod Pests<br />
<strong>and</strong> Insect Borne Diseases, Integrated Management of Plant Pests <strong>and</strong> Diseases 5,<br />
DOI 10.1007/978-90-481-8606-8_11, © Springer Science+Business Media B.V. 2010
250<br />
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reproductive potential of mites makes many acarine species ideal model <strong>org</strong>anisms<br />
for detailed epidemiological investigations.<br />
Pathogens in populations of mite species often play a major role in the<br />
regulation of population size <strong>and</strong> population density in natural habitats. In several<br />
instances, we see that populations of pest species in agricultural systems are kept<br />
below the economic threshold level <strong>by</strong> the occurrence of a disease. Such<br />
observations often provide impetus for further studies on the pathogen involved that<br />
may eventually lead to the successful application of a pathogen for the biological<br />
control of a mite pest. In addition, the occurrence of disease may be undesirable, e.g.<br />
in the case of cultures of beneficial mites: several cases have been reported on the<br />
occurrence of disease in mass cultures of predatory mites. In many instances, such<br />
observations have led to comprehensive studies on the mite pathogen involved.<br />
Interest in pathogens of mites is increasing. This is apparent from literature<br />
reviews that have been published in recent years. We refer to reviews <strong>by</strong> Van der<br />
Geest (1985), McCoy (1996), Poinar <strong>and</strong> Poinar (1998), Samish <strong>and</strong> Řeháček<br />
(1999), Ch<strong>and</strong>ler et al. (2000) <strong>and</strong> Van der Geest, Elliot, Breeuwer, <strong>and</strong> Beerling<br />
(2000). A survey of pathogenic fungi infecting plant-inhabiting mites can be found<br />
in Van der Geest (2004). The student is referred to these reviews if more detailed<br />
information is required than is given in the underlying chapter.<br />
Mites obtain their food in general <strong>by</strong> inserting their mouth parts into their<br />
vertebrate host or plant tissue. It is therefore unlikely that mites would contract<br />
disease through the alimentary tract unless the vertebrate host or food plant is<br />
infected <strong>by</strong> a pathogen. As penetration through the mouth parts is hampered, the<br />
pathogen should follow other infection routes. A plausible infection route is through<br />
the integument. Fungi are in general capable to penetrate a mite (or other arthropod<br />
species) through the integument. It is therefore not surprising that most mite<br />
pathogens are found among the fungi.<br />
In this chapter, the different groups of micro<strong>org</strong>anisms that may cause diseases<br />
in Acari will be treated.<br />
2. VIRUS DISEASES<br />
Relatively few viruses are known from mites, in strong contrast to what is observed<br />
in insects, from which more than 1,600 viruses have been described in about 1,100<br />
species. Insect viruses are often embedded in larger inclusion bodies, as is the case<br />
for nuclear polyhedrosis viruses. The rod-shaped virus particles are situated in<br />
proteinaceous bodies that protect the virus against unfavorable conditions when<br />
released from the insect cadaver. Such structures are not found for viruses that are<br />
known from mites. Well-studied viruses in mites are found in two spider mite<br />
species: the citrus red mite, Panonychus citri, <strong>and</strong> the European red mite, P. ulmi.<br />
The first record on a virus disease in a spider mite is <strong>by</strong> Muma (1955), who<br />
noted diseased mites in a natural population of the citrus red mite (CRM) in Florida,<br />
USA. Affected mites showed signs of diarrhea <strong>and</strong> the cadavers were adhered to the<br />
leaf surface <strong>by</strong> a black resinous material that was excreted from the anus. The<br />
disease has later also been reported in California <strong>by</strong> Smith, Hill, Munger, <strong>and</strong>
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251<br />
Gilmore (1959). They observed spherical particles inside diseased mites <strong>and</strong><br />
assumed that these were virus particles. Later, it could be demonstrated that a rodshaped,<br />
non-inclusion virus is the cause of the disease (Reed & Hall, 1972). The<br />
virus particles are approximately 194 × 58 nm in size <strong>and</strong> enclosed in an envelope of<br />
circa. 266 × 111 nm. The virus is formed inside the nuclei of epithelial cells of the<br />
midgut, but later it moves out of the nucleus, into the cytoplasm. The pathogen is<br />
transmitted when healthy mites ingest the feces of infected mites.<br />
The spherical particles were studied in more detail <strong>by</strong> Reed <strong>and</strong> Desjardins<br />
(1978). These authors found spherical particles of three different sizes, but only in<br />
laboratory reared mites. The particles were apparently acquired <strong>by</strong> the mites from<br />
the green lemons on which they were grown. No detrimental effects of the particles<br />
on the mites were observed, although the spheres did multiply inside the mites. In<br />
diseased mites, birefringent bodies of irregular shape were found. The size of these<br />
bodies may vary from a few micrometers up to 50 μm in diameter (Smith &<br />
Cressman, 1962). The function of these bodies is not known, but they seem to be<br />
associated with the formation of the so-called fecal pellets, that probably contain<br />
guanine as excretion product. Similar bodies have been found in mites showing poor<br />
physiological condition (see Section 6.1).<br />
The virus disease is common in citrus groves in California <strong>and</strong> Arizona <strong>and</strong><br />
causes a considerable reduction in the population density of the CRM (Reed, 1981).<br />
In the 1960s, efforts were made to use the virus as a biological acaricide in order to<br />
control the CRM. A drawback in the use of viruses for biological control is that<br />
multiplication is only possible in living cells. Control experiments were carried out<br />
<strong>by</strong> spraying aqueous suspensions of macerated diseased mites (Shaw, Chambers, &<br />
Tashiro, 1968). For this purpose, mites were grown on green lemons <strong>and</strong> harvested<br />
after infection. This is a very laborious method <strong>and</strong> can only be done for small field<br />
experiments. Another more efficient method was the collection of infected mites in<br />
the field <strong>by</strong> means of a vacuum-suction devise. The mites were subsequently kept on<br />
lemons for an additional 6–7 days in order to increase the level of infection.<br />
Application of field collected material usually rendered better results than virus<br />
suspensions obtained from laboratory cultured mites. The results in small field trials<br />
were promising, but large field applications were less satisfactory. Reasons are that<br />
the virus is easily inactivated <strong>by</strong> sunlight when applied as an aqueous suspension<br />
<strong>and</strong> that high temperatures have a negative effect on the virulence of the pathogen.<br />
An advantage of using viruses as biological control agent is that they have a narrow<br />
host spectrum: they are able to infect only a few species of spider mite <strong>and</strong> show no<br />
effect on other <strong>org</strong>anisms, e.g. phytoseiids (Shaw, Moffitt, & Sciven, 1967).<br />
Steinhaus (1959) studied a virus disease of the European red mite (ERM) in<br />
California. He observed spherical particles with a size of 40–60 nm inside affected<br />
mites <strong>and</strong> assumed that these were virus particles. A virus disease was also observed<br />
in P. ulmi in fruit orchards in Ontario (Putman & Herne, 1966). This disease was<br />
caused <strong>by</strong> a rod-shaped virus that developed inside the nuclei of fat body cells.<br />
There is no conclusive evidence that we are dealing with the same virus as the one<br />
that described from California. Affected mites can be recognized <strong>by</strong> a darker color<br />
of the immature stages, but diseased adults show no difference in color. The most<br />
conspicuous symptoms, however, is the presence of birefringent bodies inside the
252<br />
L.P.S. VAN DER GEEST<br />
midgut of the mites. These crystal-like structures probably contain guanine. The virus<br />
may cause epizootics in natural populations, but only at high densities of the spider<br />
mite. Field experiments were carried out <strong>by</strong> Putman (1970) <strong>by</strong> introducing infected<br />
immature mites into a peach orchard. In this way, a considerable reduction of the mite<br />
population could be obtained. Sprays of aqueous suspensions of the virus were less<br />
successful. It was assumed that the leaves release virus inhibitors that inactivate the<br />
virus. Recent studies on virus diseases in tetranychids have not been conducted.<br />
Transmission electron microscopy (TEM) has revealed virus-like particles in<br />
diseased females of the predatory mite Metaseiulus occidentalis (Poinar & Poinar,<br />
1998). Diseased females in laboratory colonies showed a reduced oviposition <strong>and</strong><br />
often died suddenly with a paralyzed appearance (Hoy & Jeyaprakash, 2008). Three<br />
types of icosahedral virus particles were detected <strong>by</strong> TEM analysis. One type was<br />
situated in epithelial cells, 47 nm in diameter with an electron dense core of 35 nm.<br />
Poinar <strong>and</strong> Poinar (1998) assumed that these particles were similar to those reported<br />
earlier in the citrus red mite <strong>and</strong> also similar to those found in epithelial cells of<br />
diseased <strong>and</strong> healthy twospotted spider mites (see above). It might be possible that<br />
the predatory mites obtained these particles from their prey, T. urticae. A second<br />
type of virus particles in M. occidentalis was approximately 38 nm in diameter with<br />
an electron dense core of 20 nm. These particles were located in large numbers in<br />
the nuclei of midgut cells, but free virions were also observed in the cytoplasm <strong>and</strong><br />
lumen of the midgut. A third type of virus particles was 45 nm in diameter with a 35<br />
nm dense core. These particles were only observed in tissue of the alimentary tract.<br />
We know little about the etiology of the disease <strong>and</strong> whether these observed<br />
particles are the cause of the disease <strong>and</strong> whether the predator becomes infected <strong>by</strong><br />
feeding on infected prey. The predatory mites studied belonged to crowded<br />
laboratory colonies, no field material had been included in the study.<br />
Virus-like particles have been observed in the yolk of eggs developing inside gravid<br />
Neoseiulus cucumeris <strong>by</strong> Steiner (1993) <strong>and</strong> inside Phytoseiulus persimilis females <strong>by</strong><br />
Bjørnson, Steiner, & Keddie (1997). In adults of these species, also birefringent crystals<br />
were observed, but there may be no relation between the presence of the virus-like<br />
particles <strong>and</strong> these crystals.Virus infections in cultures of predatory mites are undesirable<br />
as such conditions may affect the efficacy of the predator as biological control agent.<br />
Several phytophagous species are known to transmit plant viruses. For example, the<br />
dry bulb mite Aceria tulipae has been reported as vector of two viruses of Allium sp.<br />
(Van Dijk & Van der Vlugt, 1994) <strong>and</strong> Brevipalpus spp. are known as vector of, among<br />
others, citrus leprosis virus in citrus in Latin America (Rodrigues, Kitajima, Childers, &<br />
Chagas, 2003), of orchid fleck virus in many orchid species world-wide (Kondo, Maeda,<br />
& Tamada, 2003) <strong>and</strong> of coffee ringspot virus in coffee in Brazil <strong>and</strong> Costa Rica<br />
(Chagas, Kitajima, & Rodrigues, 2003). It is doubtful whether these vector mites suffer<br />
from the presence of viruses inside their body, although the high plain virus <strong>and</strong> Pigeon<br />
Pea Mosaic virus seem to replicate in their respective vectors (Kumar, Duncan, Robert,<br />
Jones, & Reddy, 2002). The Brome Mosaic Virus, usually transmitted <strong>by</strong> a beetle, is<br />
capable to multiply in the eriophyid Aceria tulipae. It may cause severe cytopathological<br />
effects in the midgut cells of the mite (Paliwal, 1972). Similarly, mites e.g.<br />
Dermanyssoidea play a role in the transmission of viruses to vertebrates (e.g. equine<br />
encephalitis viruses, West Nile virus, fowl pox virus) (Valiente Moro, Chauve, &
MITE PATHOGENS IN IPM<br />
253<br />
Zenner, 2005). It is not within the scope of this article to describe these viruses<br />
comprehensively, as they are considered to be plant, resp. vertebrate viruses.<br />
Several viruses are known from the honeybee (Apis mellifera), some of which<br />
are associated with the varroa mite Varroa jacobsoni <strong>and</strong> the honeybee tracheal mite<br />
(HBTM) Acarapis woodi (Sammataro, Gerson, & Needham 2000). These viruses<br />
may always be present in the bee, either in a latent or in an unapparent form.<br />
Wounds inflicted <strong>by</strong> the mites may activate the viruses in the bee. These viruses are<br />
probably not capable to infect the varroa mite or the HBTM, but the presence of<br />
these mites affects the incidence of virus disease in honey bees. The varroa mite may<br />
also play a role in the transmission of Bee Kashmir Virus (KBV), although the virus<br />
was already known from bee colonies before Apis mellifera colonies were infested<br />
<strong>by</strong> V. destructor. The presence of the virus in the mite has been demonstrated <strong>by</strong><br />
several authors (e.g. Chen, Pettis, Evans, Kramer, & Feldlaufer, 2004). Virus-free<br />
mites may become infected <strong>by</strong> coinhabiting in the same cell as virus-infected mites.<br />
Whether transmission to honey bees occurs mechanically or biologically is a<br />
question that has not yet been conclusively solved. Shen, Yang, Cox-Foster, <strong>and</strong> Cui<br />
(2005) suggested that varroa mites cause suppression of the immune system of the<br />
honey been which leads to activation of latent virus infections.<br />
Liu (1991) found virus-like particles in a sample of HBTM that originated from<br />
Scotl<strong>and</strong>, but no such particles were found in HBTM samples from California.<br />
Tissues of affected mites showed extensive lysis, while most cells were tightly<br />
packed with virus-like particles. The virions are 27–30 nm in size <strong>and</strong> are arranged<br />
in paracrystalline arrays forming hexagonal patterns. The ultrastructural morphology<br />
of the particles indicates that we may be dealing with a picorna-like virus. Such<br />
viruses resemble picornaviruses that are found in vertebrates. Picorna-like viruses<br />
are also known from honeybees, but on the basis of histopathological studies it was<br />
assumed that the virus found in HBTM is not derived from honeybees, but actually<br />
multiplies inside the mite.<br />
Kleespies, Radtke, <strong>and</strong> Bienefield (2000) performed a search for diseases in<br />
varroa mites in parasitized bee colonies. They found mites with characteristic<br />
internal black-colored changes of the gut <strong>and</strong> the fat body. On living adult bees,<br />
3.6% of the mites showed this anomaly, in brood cells, even 8% of the juvenile<br />
mites were affected. Disease incidence <strong>and</strong> intensity of the symptoms can be<br />
enhanced <strong>by</strong> changes in environmental conditions, such as deficiency of bee brood,<br />
deficiency of pollen, abnormal brood temperature <strong>and</strong> death of the host. The authors<br />
found that longevity of black-colored mites was reduced <strong>by</strong> 43%. Cytopathological<br />
studies showed the presence of a large number of spherical virus-like particles,<br />
especially in the nuclei of fatbody <strong>and</strong> muscle tissue. The particles measure<br />
approximately 27–60 nm in diameter <strong>and</strong> were very similar to the particles found <strong>by</strong><br />
Liu (1991) in HBTM. Per os infection experiments with extracts of fatbody tissue<br />
derived from symptomatic mites were unsuccessful.<br />
Ongus et al. (2004) detected virus-like particles in varroa mites that were<br />
collected in bee hives in The Netherl<strong>and</strong>s. The virions were mainly present in the<br />
cytoplasm of mite tissue <strong>and</strong> resemble the virus-like particles found <strong>by</strong> Kleespies<br />
et al. (2000). Immunochemical studies revealed that the virus was localized in the<br />
abdominal part of the alimentary tract <strong>and</strong> in the gastric caeca, but not in the salivary
254<br />
L.P.S. VAN DER GEEST<br />
gl<strong>and</strong>s (Ongus, 2006). It was possible to isolate the virus <strong>and</strong> to determine the base<br />
sequence of the virus genome. The virus (Varroa destructor virus 1) is a single<br />
str<strong>and</strong>ed RNA genome <strong>and</strong>, based on the base sequence, it was decided that it belongs<br />
to the genus Iflavirus (Ongus et al., 2004). Viruses in this genus belong also to the<br />
picorna-like viruses. The virus is closely related to deformed wing virus, known from<br />
honey bees. The latter virus causes morphological anomalies in wings of bees.<br />
3. DISEASES CAUSED BY BACTERIA<br />
The most widely studied bacterium in invertebrate pathology is Bacillus<br />
thuringiensis. It was first described in 1915 <strong>by</strong> Berliner, who isolated it from soil<br />
samples in the Thuringian Forest in Germany. Simultaneously with spore formation,<br />
a crystalline body is formed in the bacterium. Upon ingestion <strong>by</strong> an insect, this<br />
crystal (δ-endotoxin) falls apart into toxic subunits that may cause paralysis of the<br />
alimentary tract, resulting in the death of the insect. Most varieties (serotypes) of B.<br />
thuringiensis show an effect on larvae of Lepidoptera, but some also on other groups<br />
of insects, e.g. Coleoptera <strong>and</strong> Diptera.<br />
Very comprehensive research has been carried out on B. thuringiensis that has<br />
resulted in the development of several commercial preparations that are mainly used<br />
against lepidopterous pests. Also, the gene encoding for the crystalline toxic body<br />
has been isolated <strong>and</strong> transferred into crop plants, e.g. corn <strong>and</strong> cotton, making these<br />
crops resistant towards a number of lepidopterous pests. Several serotypes of B.<br />
thuringiensis produce in addition an exotoxin, the β-exotoxin, named thuringiensin.<br />
This exotoxin is excreted <strong>by</strong> the bacterium into the culture medium. It has a<br />
nucleotide-like structure <strong>and</strong> inhibits DNA-dependent RNA polymerase. This results<br />
in a blockage of mitosis. When thuringiensin is applied to young holometabolous<br />
insects, morphological deformations may occur in the adult stage.<br />
Field applications of thuringiensin were successful against the citrus red mite P.<br />
citri (Hall, Hunter, & Arakawa, 1971) <strong>and</strong> Tetranychus pacificus (Hoy & Ouyang,<br />
1987). Later, Royalty, Hall, <strong>and</strong> Taylor (1990) conducted experiments <strong>by</strong> testing two<br />
different formulations of thuringiensin against the twospotted spider mite T. urticae.<br />
The results indicated that thuringiensin might be a potential acaricide. In particular<br />
young instars are susceptible, since these have a high growth rate. Various<br />
physiological processes in young <strong>org</strong>anisms require higher RNA synthesis than in<br />
the older slower growing stages. A major drawback is that thuringiensin is toxic for<br />
a wide range of <strong>org</strong>anisms. Not only are spider mites affected, but also beneficial<br />
mites, such as Phytoseiulus persimilis: oviposition starts to decline after 2 days <strong>and</strong><br />
ceases completely after 3–4 days in both predator <strong>and</strong> spider mite T. urticae (Guo,<br />
Zuo, Zhao, Wang, & Jiang, 1993). The chemical is apparently a nonselective<br />
acaricide that should not be used in combination with predatory mites.<br />
The spore-crystal complex of B. thuringiensis has been tested on spider mites<br />
<strong>by</strong> Krieg (1972), but no mortality was observed. However, Chapman <strong>and</strong> Hoy<br />
(1991) conducted experiments in which T. urticae <strong>and</strong> Metaseiulus occidentalis<br />
were treated with a commercial preparation of B. thuringiensis var. tenebrionis. This<br />
variety of B. thuringiensis shows an effect on beetles <strong>and</strong> is recommended for use<br />
against the Colorado Potato Beetle, Leptinotarsa decemlineata. No effect was noted
MITE PATHOGENS IN IPM<br />
255<br />
on the twospotted spider mite, but the preparation did show a toxic effect on M.<br />
occidentalis. Eggs were not affected, but if juveniles were treated, only 65% reached<br />
the adult stage. This toxic effect could be enhanced <strong>by</strong> starving the mites: the<br />
authors assumed that starvation may lead to a higher uptake of the material, or that<br />
the mites were more exposed to the preparation as starving mites tend to move<br />
faster. It is also possible that starvation acts as a stress factor. The authors have no<br />
explanation for the toxic effect on the predatory mite: the preparation did not contain<br />
the β-exotoxin (thuringiensin) known to be toxic for mites.<br />
In more recent years, isolates of B. thuringiensis have been found that do show<br />
toxicity towards spider mites <strong>and</strong> house dust mites (Payne, Cannon, & Bagley, 1993;<br />
Payne, Cannon, & Ralph, 1994). It has been suggested to isolate the δ-endotoxin of these<br />
isolates <strong>and</strong> to formulate it as an acaricide. One may also transfer the gene, encoding for<br />
this specific δ-endotoxin into a crop plant in order to protect the crop against spider mite<br />
infestations.<br />
An interesting discovery is the isolation of a B. thuringiensis strain from dead<br />
twospotted spider mites, T. urticae (Jung, Mizuki, Akao, & Côte, 2007). In<br />
sporulating cultures of the bacterium, roughly spherical parasporal inclusion bodies<br />
are formed. This crystalline body is composed of at least two polypeptides of 86 <strong>and</strong><br />
79 KDa. The crystal is not toxic to the twospotted spider mite, but after cleavage<br />
with trypsin, it is cytocidal to some human cancer cells.<br />
In Table 1, a list is given of bacteria that have been isolated from mites. We realize<br />
that this list may not be complete, but we have tried to limit the list to bacteria that show<br />
pathogenicity towards mites. Many species of bacteria may be isolated from mites (<strong>and</strong><br />
other <strong>org</strong>anisms): in many instances, these may not appear to be pathogenic.<br />
Aksoy, Ozman-Sullival, Ocal, Celik, <strong>and</strong> Sullivan (2008) studied the effect of<br />
Pseudomonas putida biotype B on the twospotted spider mite T. urticae. The<br />
bacterium had been isolated from greenhouse soil in Turkey <strong>and</strong> was tested on newly<br />
emerged, copulated females. The authors observed a strongly reduced egg production<br />
<strong>and</strong> no hatching of the eggs was noted. The results showed that the bacterium may be<br />
very effective in causing mortality in T. urticae populations. Further research is<br />
required to find out whether this <strong>org</strong>anism may be developed to a microbial miticide.<br />
The predatory mite Phytoseiulus persimilis has been mass cultured for several<br />
decades for the biological control of spider mites in various field <strong>and</strong> glasshouse crops.<br />
This predator species is very important in integrated pest control programs <strong>and</strong> has<br />
stimulated research on predator-prey interactions <strong>and</strong> foraging behavior. It has been<br />
shown in several instances that adult female predatory mites are attracted to volatiles that<br />
are emitted <strong>by</strong> plants infested <strong>by</strong> prey. This emission of volatiles <strong>by</strong> the plant after<br />
herbivore attack is apparently a defense mechanism against herbivorous mites. Schütte<br />
(2006) noticed a change in response to prey-induced plant volatiles in a laboratory<br />
colony of P. persimilis. This population showed a lower attraction to these volatiles than<br />
other populations of the predator. It could be demonstrated that the change in behavior is<br />
caused <strong>by</strong> the involvement of a bacterium. Transmission of the bacterium occurs through<br />
feces <strong>and</strong> debris. There is no evidence that vertical transmission (from one generation to<br />
the next) occurs. The bacterium could be isolated <strong>and</strong> was described as Acaricomes<br />
phytoseiuli (Pukall, Schumann, Schütte, Gols, & Dicke, 2006). Comparative analysis of<br />
the 16S rDNA sequence revealed that it belongs to the Micrococcaceae, <strong>and</strong> that it is
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L.P.S. VAN DER GEEST<br />
related to the soil bacterium Arthrobacter globiformis, to A. rissicus, a bacterium<br />
originally isolated from air in the Russian space laboratory <strong>and</strong> to Renibacterium<br />
salmoninarum, the causal agent of kidney disease in salmon. The bacterium clearly<br />
affects the effectiveness of P. persimilis as biological control agent as infected mites<br />
show a lower response to the volatiles emitted <strong>by</strong> the plant after herbivorous attack. At<br />
this moment, there are no signs that the disease is present in commercial populations of<br />
P. persimilis, nor is it widespread in laboratory populations of this predator.<br />
Table 1. Bacterial infections in mites.<br />
Species Mite host Mite family References<br />
Bacillus<br />
thuringiensis<br />
Spider mites<br />
House dust mites<br />
Tetranychidae<br />
Pyroglyphidae<br />
Payne et al. (1993, 1994)<br />
B. thuringiensis Tetranychus urticae Tetranychidae Jung et al. (2007)<br />
B. thuringiensis<br />
var. israelensis<br />
Dermatophagoides<br />
pteronyssinus<br />
Pyroglyphidae Saleh et al. (1991)<br />
B. thuringiensis<br />
var. tenebrionis<br />
Metaseiulus occidentalis Phytoseiidae Chapman <strong>and</strong> Hoy (1991)<br />
B. sphaericus Dermatophagoides<br />
pteronyssinus<br />
Pyroglyphidae<br />
Saleh, Kelada <strong>and</strong> Shader<br />
(1991)<br />
Bacteroidetes Metaseiulus occidentalis Phytoseiidae Hoy <strong>and</strong> Jeyaprakash (2008)<br />
Enterobacter Metaseiulus occidentalis Phytoseiidae Hoy <strong>and</strong> Jeyaprakash (2008)<br />
Pseudomonas<br />
putida<br />
Acaricomes<br />
phytoseiuli<br />
Tetranychus urticae Tetranychidae Aksoy et al. (2008)<br />
Phytoseiulus persimilis Phytoseiidae Pukall et al. (2006).<br />
Rickettsia sp. Metaseiulus occidentalis Phytoseiidae Hess <strong>and</strong> Hoy (1982)<br />
Vatacarus ipoides Trombiculidae Thomas <strong>and</strong> Poinar (1973)<br />
Rickettsiella<br />
phytoseiuli<br />
Phytoseiulus persimilis Phytoseiidae Šut’áková (1988)<br />
Wolbachia Bryobia sp. Tetranychidae Weeks (personal<br />
communication)<br />
Eutetranychus orientalis Tetranychidae Breeuwer <strong>and</strong> Jacobs (1996)<br />
Oligonychus biharensis Tetranychidae Breeuwer <strong>and</strong> Jacobs (1996)<br />
Tetranychus yusti Tetranychidae Breeuwer <strong>and</strong> Jacobs (1996)<br />
Tetranychus kanzawai Tetranychidae Breeuwer <strong>and</strong> Jacobs (1996)<br />
Gomi, Gotoh, <strong>and</strong> Noda (1997)
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257<br />
Table 1 Continued<br />
Tetranychus<br />
neocaledonicus<br />
Tetranychidae Breeuwer <strong>and</strong> Jacobs (1996)<br />
Tetranychus turkestani Tetranychidae Breeuwer <strong>and</strong> Jacobs (1996)<br />
Tetranychus quercivorus Tetranychidae Gotoh, Abe, Kurihara, <strong>and</strong><br />
Suzuki (1995)<br />
Tetranychus urticae Tetranychidae Breeuwer <strong>and</strong> Jacobs (1996)<br />
Tsagkarakou, Guillemaud,<br />
Rousset, <strong>and</strong> Navajas (1996)<br />
Metaseiulus occidentalis Phytoseiidae Johanowicz <strong>and</strong> Hoy (1966)<br />
Breeuwer <strong>and</strong> Jacobs (1996)<br />
Neoseiulus barkeri Phytoseiidae Breeuwer <strong>and</strong> Jacobs (1996)<br />
Neoseiulus bibens Phytoseiidae Breeuwer <strong>and</strong> Jacobs (1996)<br />
Phytoseiulus persimilis Phytoseiidae Steiner (1993) <strong>and</strong> Breeuwer<br />
<strong>and</strong> Jacobs (1996)<br />
Cardinium sp.<br />
Brevipalpus phoenici<br />
Brevipalpus californicus<br />
Euseius finl<strong>and</strong>icus<br />
Neoseiulus californicus<br />
Metaseiulus occidentalis<br />
Tenuipalpidae<br />
Tenuipalpidae<br />
Phytoseiidae<br />
Groot <strong>and</strong> Breeuwer (2006)<br />
Chigira <strong>and</strong> Miura (2005)<br />
Enigi <strong>and</strong> Schausberger<br />
(2007) Hoy <strong>and</strong> Jeyaprakash<br />
(2008)<br />
Spiroplasma<br />
Tetranychus urticae<br />
Dermanyssus gallinae<br />
Tetranychidae<br />
Dermanyssidae<br />
Enigi <strong>and</strong> Schausberger (2007),<br />
De Luna, Valente Moro, Guy,<br />
Zenner, <strong>and</strong> Sparagano (2009)<br />
Serratia<br />
marcescens<br />
Metaseiulus occidentalis Phytoseiidae Lighthart, Sewall, <strong>and</strong><br />
Thomas (1988)<br />
Mite <strong>and</strong> also tick species are frequently infected with intra-cellular<br />
micro<strong>org</strong>anisms (Šut’áková, 1988, 1994; Steiner, 1993; Munderloh & Kurtti, 1995;<br />
Bjørnson et al., 1997) These micro<strong>org</strong>anisms have been placed into the family<br />
Rickettsiaceae within the class α-Proteobacteria. The family Rickettsiaceae (or<br />
Rickettsia-like <strong>org</strong>anisms) consists of three tribes: Rickettsieae, Ehrlichieae <strong>and</strong><br />
Wolbachieae (Weiss & Moulder, 1984). Representatives of these tribes have a number<br />
of features in common: they are obligate intracellular gram-negative bacteria naturally<br />
found in arthropod hosts, they multiply inside eukaryotic cells <strong>and</strong> are often<br />
surrounded <strong>by</strong> multiple membranes. Some are also capable of infecting humans <strong>and</strong><br />
other vertebrates <strong>and</strong> are frequently pathogenic in these secondary hosts They often<br />
cause severe diseases such as spotted fever, typhus <strong>and</strong> scrub typhus (Hayes &<br />
Burgdorfer, 1989). A good classification of these <strong>org</strong>anisms has been hampered <strong>by</strong> the<br />
fact that classical microbiological identification tools cannot be used because of their
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L.P.S. VAN DER GEEST<br />
obligate intracellular lifestyle. Since a number of years, tools have become available to<br />
sequence DNA of <strong>org</strong>anisms. Sequence information on 16S rDNA genes has revealed<br />
interesting aspects of the order Rickettsiales, including their phylogeny. For additional<br />
information see Van der Geest et al. (2000).<br />
The best studied group of rickettsia are those that are vectored <strong>by</strong> ticks, as they<br />
often cause disease in vertebrates <strong>and</strong> are therefore of great medical <strong>and</strong> veterinary<br />
importance. In plant-inhabiting mites, rickettsia-like infections have mainly been<br />
observed in microscopic surveys (Šut’áková, 1988, 1994; Hess & Hoy, 1982;<br />
Steiner, 1993; Munderloh & Kurtti, 1995; Bjørnson et al., 1997). They are described<br />
as intracellular microbes often localized in the reproductive tissue of their host, but<br />
no data are available on their possible effect on mites.<br />
Hess <strong>and</strong> Hoy (1982) studied diseased laboratory colonies of the predatory mite<br />
Metaseiulus occidentalis more comprehensively, as these colonies produced only<br />
few eggs <strong>and</strong> often died out. Two different pathologies could be discerned. Some<br />
adult females were plump in appearance <strong>and</strong> had cream- to pink-colored plugs<br />
excreting from their rectum. Such females rarely produced eggs, although they<br />
appeared gravid. Immatures <strong>and</strong> males seldom showed this plug. The second<br />
condition affected both females <strong>and</strong> juveniles. These females failed to lay eggs <strong>and</strong><br />
immatures often died, in particular during molting. Two forms of Rickettsia-like<br />
<strong>org</strong>anisms were described, based on structure of the cell wall <strong>and</strong> the presence of<br />
cytoplasmic inclusions. Type A was observed in all mites examined, while type B<br />
was present in approximately two-thirds of the mites investigated. The Type A<br />
<strong>org</strong>anisms were small, ovoid <strong>and</strong> 0.75 μm in length <strong>and</strong> 0.5 μm in width, with a<br />
trilaminar membrane of 7 nm thick, while Type B was rod-shaped, <strong>and</strong> measured 0.5<br />
μm in width <strong>and</strong> 2 μm in length. The Type A <strong>org</strong>anisms were located intracellularly,<br />
singly or in groups of two or three in all tissues except ovarian <strong>and</strong> nervous tissue.<br />
The Type B <strong>org</strong>anisms were both inter-<strong>and</strong> extracellular within membrane-bound<br />
vacuoles of cells that are similar in structure to mycetomes in insects. For a more<br />
detailed description is referred to Hoy <strong>and</strong> Jeyaprakash (2008).<br />
Since the mid-1990s, molecular screening for intracellular micro<strong>org</strong>anisms is<br />
possible. This has resulted in the discovery of Wolbachia in tetranychid <strong>and</strong><br />
phytoseiid mites (e.g. Gotoh et al. 1995; Gotoh, Gomi, & Nagata, 1999; Gotoh,<br />
Sugasawa, & Nagata, 1999; Breeuwer & Jacobs, 1996; Johanowicz & Hoy, 1996;<br />
Tsagkarakou et al., 1996). Probably all Rickettsia-like <strong>org</strong>anisms that have been<br />
reported in the early microscopic surveys are members of the genus Wolbachia<br />
belonging to the family Rickettsiaceae. These bacteria are parasites of the<br />
reproductive system of mites <strong>and</strong> insects <strong>and</strong> cause many unusual effects in their<br />
hosts, such as parthenogenesis (infected females produce only females), male killing<br />
(male embryos die while female embryos develop into adults), feminization<br />
(infected male embryo’s develop into females) <strong>and</strong> cytoplasmic incompatibility.<br />
Wolbachia is a bacterium that is vertically transmitted to the next generation<br />
through the females. It modifies host reproduction in several ways in order to<br />
enhance its own spread (Weeks & Breeuwer, 2001). It induces parthenogenesis in<br />
the spider mite Bryobia praetiosa, causing males not to be produced. This is to the<br />
advantage of the bacterium, as only females are able to transmit the pathogen to the
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259<br />
next generation. Probably over 1 million species of insects are infected, <strong>and</strong><br />
infection rates in other taxa of arthropods may be similar.<br />
Van Opijnen <strong>and</strong> Breeuwer (1999) showed that Wolbachia can induce<br />
cytoplasmic incompatibility in the arrhenotokous 1 twospotted spider mite<br />
Tetranychus urticae between uninfected females <strong>and</strong> infected males.<br />
Cytoplasmic incompatibility is expressed through a male-biased sex ratio <strong>and</strong><br />
low hatchability of eggs. It could be suppressed <strong>by</strong> removing Wolbachia from<br />
spider mites reared on a diet with antibiotics. The authors also demonstrated that<br />
heat treatment (32° C.) can eliminate Wolbachia from infected mites. It was<br />
shown that 71% of the mites were “cured” after being reared for four<br />
generations at 32°C. The infection could be completely eliminated <strong>by</strong> keeping<br />
the mites for 6 generations at 32°C.<br />
In a recent study Hoy <strong>and</strong> Jeyaprakash (2008) studied M. occidentalis females<br />
with large anal plugs. These females were collected from crowded laboratory<br />
colonies. The authors used 16S PCR primers to amplify the bacterial DNA <strong>and</strong><br />
subsequently cloned <strong>and</strong> sequenced the products. It was remarkable that only<br />
bacteria were found that could also be detected in “healthy” females, viz. Wolbachia,<br />
Cardinium, an undescribed species of Bacteroidetes <strong>and</strong> an Enterobacter species.<br />
The authors assumed that stress could increase the titer of one or more<br />
endosymbionts which may lead to “disease”. The authors cite the statement of Dale<br />
<strong>and</strong> Moran (2006) that “as more cases of chronic bacterial infection are<br />
characterized, the distinction between pathogenesis <strong>and</strong> mutualism has become<br />
increasingly blurred. Infection <strong>by</strong> a particular bacterium may be beneficial to a host<br />
under circumstances but harmful in other hosts or environments” Another<br />
interpretation for the occurrence of the disease in M. occidentalis is that the predator<br />
obtains Rickettsia-like <strong>org</strong>anisms from its food. Rickettsia-like <strong>org</strong>anisms have been<br />
detected in twospotted spider mites. However, there is no conclusive evidence that<br />
the predator obtains the endosymbionts from its prey (Hoy & Jeyaprakash, 2008).<br />
Groot <strong>and</strong> Breeuwer (2006) showed the presence of the symbiont Cardinium in<br />
the thelytokous 2 mite species Brevipalpus phoenici. Cardinium spp. belong to the<br />
Flexibacteraceae (Phylum: Bacteroidetes; Class: Sphingobacteria). It was<br />
demonstrated that Cardinium induces thelytoky <strong>by</strong> feminizing unfertilized haploid<br />
eggs. Isofemale lines were set up <strong>and</strong> in some of these lines, males were produced<br />
<strong>by</strong> only very young daughters, while older females produce daughters exclusively.<br />
That a bacterium was involved was apparent from the fact that a treatment with<br />
antibiotics resulted in an increased number of male progeny. The presence of<br />
Cardinium was also shown in B. californicus (Chigira & Miura, 2005). Tetracyclinetreated<br />
females produced many male progeny while untreated females produced<br />
only female progeny. This is an indication that B. californicus is feminized <strong>by</strong><br />
Cardinium. Comparison of infected females with uninfected males <strong>and</strong> other closely<br />
related species, revealed that Cardinium does not have a negative effect on the<br />
fitness of B. californicus. The bacterium has also been found in a population of<br />
1 Arrhenotokous: capable of producing male offspring only.<br />
2 Thelytokous: capable of producing female offspring only.
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L.P.S. VAN DER GEEST<br />
Eotetranychus suginamensis in Japan (Gotoh, Noda, & Ito, 2006). One species of<br />
spider mite, Eotetranychus pueraricola harbored both Cardinium <strong>and</strong> Wolbachia,<br />
but these symbionts seemed to have no effect on the reproduction of the host.<br />
Cardinium has also been found to play a role in insect species, e.g. Encarsia sp.<br />
Cardinium is also present in field populations of the predatory mites Euseius<br />
finl<strong>and</strong>icus <strong>and</strong> Neoseiulus californicus <strong>and</strong> the spider mite Eotetranychus uncatus<br />
(Enigi & Schausberger, 2007). The endosymbionts has also been detected in the<br />
poultry red mite Dermanyssus gallinae (De Luna et al., 2009).<br />
Another genus of endosymbionts is the genus Spiroplasma. This genus belongs<br />
to the family Spiroplasmataceae, class Mollicutes, phylum Firmicutes. These<br />
bacteria are fastidious <strong>org</strong>anisms which means that they can only been grown on rich<br />
nutrient media. Spiroplasma has been shown to kill males of Danaus chrysippus<br />
(Lepidoptera) <strong>and</strong> also of other insect species. Interspecific transmission of<br />
Spiroplasma poulsonii, a male-killing symbiont has been demonstrated between<br />
Drosophila sp. <strong>and</strong> Macrocheles sp., an ectoparasitic mite that feeds on the<br />
hemolymph of Drosophila (Jaeniki, Polak, Fiskin, Helou, & Minhas, 2007). Enigi<br />
<strong>and</strong> Schausberger (2007) showed the presence of Spiroplasma in the twospotted<br />
spider mite, but its effect on reproduction <strong>and</strong> other biological parameters is not yet<br />
known. Spiroplasma has also been detected in the poultry red mite Dermanyssus<br />
gallinae (De Luna et al., 2009).<br />
The ecological implications of modification of reproduction in herbivorous <strong>and</strong><br />
predatory mites <strong>by</strong> intracellular symbionts is an interesting field of study. It will be<br />
clear that such modifications will have a great impact on the development of mite<br />
populations.<br />
4. DISEASES CAUSED BY FUNGI<br />
The Kingdom Fungi is a monophyletic assemblage which comprises at present four<br />
phyla: Chytridiomycota, Zygomycota, Basidiomycota <strong>and</strong> Ascomycota. In addition,<br />
there is a group called the Deuteromycetes (or Fungi Imperfecti), fungi of which no<br />
sexual stage is known. In the past, many parasitic fungi were classified in this group,<br />
but were reclassified after the sexual stage had been discovered. Most of these<br />
“reclassified” fungi belong to the Ascomycota. Nucleotide sequence analysis also<br />
suggests that the majority of these fungi belong to the Ascomycota. A large number<br />
of fungi capable to infect arthropods are found in the Deuteromycetes.<br />
Chytridiomycota <strong>and</strong> Zygomycota share common features, in particular the<br />
absence of cross walls (septa) in their hyphae. The Chytridiomycota (chytrids)<br />
represent a primitive group of aquatic fungi. Chytrids have gametes that are mobile<br />
<strong>by</strong> means of flagella. No chytrids are known that infect mites.<br />
Zygomycota are characterized <strong>by</strong> the formation of zygospores. These sexual<br />
spores are not contained within a specialized fruiting body or sac, but are unenclosed<br />
(or naked) between their parental hyphae. The haploid nuclei at the end of two<br />
hyphae fuse to a diploid zygote. This zygote undergoes immediately meiosis to form<br />
haploid cells that develop into zygospores.<br />
Ascomycota are also called “sac fungi” as their sexual spores (ascospores) are<br />
enclosed in tube-like sacs, known as asci. The formation of ascospores is similar to
MITE PATHOGENS IN IPM<br />
261<br />
that of zygospores, but the spores are not naked but contained within asci.<br />
Ascomycota have cross walls in their hyphae.<br />
Basidiomycota are also known as the “club fungi”. Their sexual spores are<br />
formed on often very complex fruiting bodies called basidia. This group of fungi<br />
possesses also septa inside their hyphae.<br />
4.1. Zygomycota<br />
In this phylum, only the order Entomomophthorales (meaning insect destroyers)<br />
(class Zygomycetes) contains species that are pathogenic for Arthropoda. These<br />
fungi are mainly obligatory pathogens of insects <strong>and</strong> other arthropods, often with a<br />
restricted host spectrum. However, some species are parasitic on desmids (green<br />
algae) or fern prothalli while other species may be saprophytic on plant debris<br />
(Moore-L<strong>and</strong>ecker, 1996). Hosts that are infected <strong>by</strong> fungi of this group are usually<br />
not killed before all available nutrients have been utilized, in contrast to, e.g.<br />
Deuteromycetes infections where mycotoxins often cause the death of the host prior<br />
to the complete utilization of food reserves. Hajek (1997) assumed that the complete<br />
utilization of the live host <strong>by</strong> the fungus seems to be consistent with the obligate<br />
nature of this group of fungi.<br />
As mentioned above, Zygomycetes are characterized <strong>by</strong> their sexual<br />
reproduction, the so-called zygospore formation, usually inside the parasitized host.<br />
Zygospores bud laterally from conjugation bridges between gametangia 3 (hyphal<br />
bodies). These thick-walled, dark-colored spores are also called resting spores <strong>and</strong><br />
may germinate to produce conidiophores with conidia attached. Other types of<br />
resting spores are chlamydospores, thick-walled, nonsexual spores originating from<br />
transformed hyphal cells, <strong>and</strong> azygospores that may arise from parthenogenetic<br />
development of hyphal bodies (short segments of mycelium inside the host).<br />
Azygospores may also be the result of budding of chlamydospores, or they may be<br />
formed at the tip of hyphae that arise from chlamydospores or hyphal bodies.<br />
Resting spores (Fig. 1) seem to aid the fungus in surviving unfavorable conditions,<br />
e.g. periods of drought. Conditions under which resting spores germinate are not<br />
well-understood.<br />
More common is the formation of sporangiospores or ballistospores. These<br />
asexual spores are nonmotile <strong>and</strong> are formed within a sac-like structure, the<br />
sporangiole. Under nearly saturated conditions, these spores (<strong>by</strong> most mycologists<br />
called: primary conidia) are forcibly discharged from the spore bearing structure<br />
(sporangiophore, conidiophore). Primary conidia are often sticky due to the presence<br />
of a mucous substance causing them to adhere to a substrate after they have been<br />
released. The conidia may either form hyphae directly that may infect a new host or<br />
form secondary conidia.<br />
Six families are recognized within the Entomomophthorales; pathogens of<br />
arthropods are mainly found in the Entomophthoraceae, Neozygitaceae <strong>and</strong><br />
Ancylistaceae. These families are recognized on the basis of nuclear characters (size,<br />
3 A single-celled structure producing gametes (sex cells) or gametic nuclei.
262<br />
L.P.S. VAN DER GEEST<br />
number, stainability), mode of formation of resting spores, <strong>and</strong> mechanism of<br />
discharge of primary conidia.<br />
Figure 1. Resting spores of Neozygites tanajoae in the cassava green mite<br />
Mononychellus tanajoa. Photograph courtesy of Dr. Fabien C.C. Hountondji.<br />
Entomophthoraceae are obligate pathogens of arthropods. In this family, primary<br />
conidia are released in a cannon-like manner when the conidiophore ruptures at the apex.<br />
The conidium is actually a bud at the apex of the conidiophore that is filled with<br />
protoplasm from the conidiophore. When the conidium is fully developed, both<br />
conidium <strong>and</strong> conidiophore absorb water quickly under humid conditions. The osmotic<br />
pressure is larger in the conidium than in the conidiophore <strong>and</strong> this fact results in the<br />
forcible discharge of the conidium. When the spore l<strong>and</strong>s on a suitable host, it may infect<br />
the host after germination. These primary conidia may form secondary conidia if l<strong>and</strong>ed<br />
on a non suitable substrate. A well-known example is Entomophthora muscae, a species<br />
capable to infect flies. Mites infecting species are known in the genus Tarichium. Of<br />
species of this genus, only resting spores are known <strong>and</strong> species determination is largely<br />
based on the shape <strong>and</strong> size of the resting spores. Tarichium spp. have been isolated in<br />
soil samples from several species of mites, in many cases Oribatidae (e.g. Bałazy &<br />
Wiśniewski, 1982, 1984).<br />
Neozygitaceae are obligate pathogens of insects (mainly Homoptera) <strong>and</strong> mites. They<br />
release primary conidia that germinate to form smaller secondary conidia with an adhesive<br />
haptor on long, thin conidiophores. The resting spores are often dark-colored <strong>and</strong><br />
ornamented on the outside wall. They possess two pores <strong>and</strong> are formed inside the hosts.<br />
Ancylistaceae contains a number of representatives that may not only infect<br />
arthropods, but also vertebrates. For example, Conidiobolus coronatus causes<br />
serious infectious of mucous membranes of humans <strong>and</strong> other vertebrates (Maiti et<br />
al., 2004). Other species in this family are found in the soil <strong>and</strong> are often<br />
saprophytic. Primary conidia are forcibly discharged towards a light source <strong>and</strong><br />
germinate to form secondary conidia that usually have the same shape as the primary<br />
conidia. The secondary conidia are either forcibly discharged or discharged<br />
passively from long slender conidiophores.
MITE PATHOGENS IN IPM<br />
263<br />
4.1.1. Course of Infection<br />
Entomophthoralean fungi usually penetrate their host through the cuticle <strong>by</strong> means<br />
of a germ tube that is formed <strong>by</strong> the conidium. Mite infecting species are mainly<br />
found in the Neozygitaceae. The primary conidium is released from the<br />
conidiophore <strong>and</strong> forms on top of a slender tube a much smaller secondary<br />
conidium, called capilliconidium. The capilliconidium is considered to be the<br />
infectious propagule. When l<strong>and</strong>ed on a suitable host, it penetrates through the<br />
cuticle <strong>by</strong> means of a newly formed germ tube (Fig. 2). After penetration, mycelium<br />
is formed within the body cavity of the host that fragments into a number of smaller<br />
segments, the hyphal bodies. Hyphal bodies are the propagative units <strong>and</strong> multiply<br />
<strong>by</strong> budding <strong>and</strong> <strong>by</strong> undergoing fission. In addition, rhizoids may be formed: sterile<br />
hyphae, often branched, that perforate the ventral side of the host <strong>and</strong> attach the host<br />
to the substrate. The infected host becomes in this way fixed to the substrate, also<br />
after its death. Favorable conditions (high relative humidity) allow the formation of<br />
conidiophores that grow through the cuticle of the host. On top of these structures,<br />
conidia are formed that form a halo around the dead host after discharge from the<br />
conidiophores. The spores have a mucous substance on the outside <strong>and</strong> stick to the<br />
substrate on which they have l<strong>and</strong>ed. They may be picked up <strong>by</strong> new, uninfected<br />
hosts. A high relative humidity (near saturation point) is required at two points in the<br />
course of the disease: germination of the spores needs a high relative humidity, but<br />
also sporulation requires humid conditions.<br />
Figure 2. Capilliconidium of a Neozygites sp. on a leg of a spider mite<br />
Photograph: Leo P.S. van der Geest.
264<br />
L.P.S. VAN DER GEEST<br />
The presence of rhizoids is an important property of the fungus for a successful<br />
transmission of the disease to a new host: the dead host (mummy) remains fixed to<br />
the plant surface <strong>and</strong> does not fall on the soil. In this way, chances for a successful<br />
transmission are increased.<br />
The formation of resting spores is an interesting phenomenon. Sometimes,<br />
resting spores are present in large numbers. It is assumed that they may assist the<br />
fungus to overcome poor favorable conditions, such as extreme periods of drought.<br />
However, we still know very little about the role of resting spores <strong>and</strong> the conditions<br />
under which they germinate are poorly understood. The fungus may also survive<br />
unfavorable conditions in other manners. Klingen, Wærsted, <strong>and</strong> Westrum (2008)<br />
showed that Neozygites floridana may survive cold winter periods in the form of<br />
hyphal bodies inside hibernating females of T.urticae.<br />
Most entomophthoralean fungi are difficult to culture in artificial culture media.<br />
For mass production, it is often necessary to use live host. Species that can be<br />
cultured in artificial media have usually a broad host spectrum. On the other h<strong>and</strong>,<br />
species with a restricted host range can hardly be grown outside their host, although<br />
some progress have been made with very complex culture media. Entomophthorales<br />
observed in mites are given in Table 2.<br />
Table 2. Entomophthoralean fungi infecting mites <strong>and</strong> their hosts.<br />
Fungus species Mite species Mite family References<br />
Not identified<br />
Entomophthoralean<br />
species<br />
Arctoseius sp.<br />
Macrocheles<br />
peregrinus<br />
Pergamasus<br />
crassipes<br />
Tetranychus<br />
desertorum<br />
Arctoseiinae<br />
Macrochelidae<br />
Parasitidae<br />
Tetranychidae<br />
Bałazy <strong>and</strong> Wiśniewski<br />
(1989)<br />
Milner (1985)<br />
Milner (1985)<br />
Walter (1999)<br />
Resting spores of<br />
Entomophtoralean<br />
species<br />
Agistemus<br />
Asca sp.<br />
Amblyseius<br />
igarassuensis<br />
Stigmaeidae<br />
Ascidae<br />
Phytoseiidae<br />
Van der Geest, De Moraes,<br />
Navia, <strong>and</strong> Tanzini (2002)<br />
Basidiobolus sp. Tetranychus urticae Tetranychidae See: Ch<strong>and</strong>ler et al. (2000)<br />
Conidiobolus sp. Bryobia sp. Tetranychidae Bałazy, Mietkiewski,<br />
Tkaczuk, Wegensteiner,<br />
<strong>and</strong> Wrzosek (2008)<br />
Conidiobolus<br />
brefeldionis<br />
Tyrophagus<br />
perniciosus<br />
Acaridae See: Ch<strong>and</strong>ler et al. (2000)<br />
Conidiobolus<br />
chapowski<br />
Pergamasus Parasitidae See: Ch<strong>and</strong>ler et al. (2000)
MITE PATHOGENS IN IPM<br />
265<br />
Table 2 Continued<br />
Conidiobolus<br />
coronatus<br />
Dendrolaelaps sp. Digamasellidae Bałazy et al. (2008)<br />
Conidiobolus<br />
obscurus<br />
Phytoseiulus<br />
persimilis<br />
Mononychellus<br />
tanajoa<br />
Tetranychus<br />
bimaculatus<br />
Tetranychus urticae<br />
Phytoseiidae<br />
Tetranychidae<br />
See: Ch<strong>and</strong>ler et al. (2000)<br />
Nyiira (1982)<br />
See: Ch<strong>and</strong>ler et al. (2000)<br />
Conidiobolus<br />
thromboides<br />
Tetranychus urticae<br />
Eotetranychus<br />
sexmaculaturs<br />
Mononychellus sp.<br />
Mononychellus<br />
tanajoa<br />
Panonychus citri<br />
Tetranychus evansi<br />
Tetranychus<br />
pacificus<br />
Tetranychus<br />
tumidus<br />
Tetranychus<br />
turkestani<br />
Vatacarus sp.<br />
Tetranychidae<br />
Trombiculidae<br />
See: Ch<strong>and</strong>ler et al. (2000)<br />
Selhime <strong>and</strong> Muma (1966)<br />
Bartkowski Odindo, <strong>and</strong><br />
Otieno (1988)<br />
Delalibera, Sosa Gomez,<br />
De Moraes, De Alencar,<br />
<strong>and</strong> Farias Araujo (1992)<br />
Fisher (1951)<br />
Humber, De Moraes, <strong>and</strong><br />
Dos Santos (1981)<br />
Steinhaus <strong>and</strong> Marsh (1962)<br />
See: Ch<strong>and</strong>ler et al. (2000)<br />
Carner <strong>and</strong> Canerday<br />
(1968)<br />
See: Ch<strong>and</strong>ler et al. (2000)<br />
Erynia<br />
phalangicidae<br />
Pergamasus sp. Parasitidae Bałazy <strong>and</strong> Wiśniewski<br />
(1984)<br />
Zoophthora radicans Tetranychus urtcae Tetranychidae See Ch<strong>and</strong>ler et al. (2000)<br />
Neozygites sp.<br />
Euseius citrifolius<br />
Alaskozetes<br />
antarcticus<br />
Phytoseiidae<br />
Ameronothridae<br />
Furtado, De Moraes, <strong>and</strong><br />
Keller (1996)<br />
Bridge <strong>and</strong> Worl<strong>and</strong> (2004,<br />
2008)<br />
Neozygites<br />
abacaridis<br />
Abacarus hystrix<br />
Aculodes mckenziei<br />
Aculodes sp.<br />
Aculus fockeui<br />
Eriophyidae<br />
Miętkiewski <strong>and</strong> Bałazy<br />
(2003)<br />
Bałazy, Mietkiewski,<br />
Tkaczuk, Wegensteiner,<br />
<strong>and</strong> Wrzosek (2008)
266<br />
L.P.S. VAN DER GEEST<br />
Table 2 Continued<br />
Neozygites acaricida<br />
Halotydeus<br />
destructor<br />
Penthaleus major<br />
Eupodidae<br />
Penthaleidae<br />
See Ch<strong>and</strong>ler et al. (2000)<br />
Neozygites acaridis<br />
Halotydeus<br />
destructor<br />
Penthaleus major<br />
Eupodidae<br />
Penthaleidae<br />
James (1994)<br />
Neozygites<br />
floridana<br />
Bryobia sp.<br />
Eotetranychus<br />
banksi<br />
Tetranychidae<br />
Miętkiewski, Balazy, <strong>and</strong> Van<br />
der Geest (1993)<br />
Weiser <strong>and</strong> Muma (1966)<br />
Oligonychus<br />
gossypii<br />
Yaninek, Saizonou, Onzo,<br />
Zannou, <strong>and</strong> Gnanvossou (1996)<br />
Oligonychus<br />
hondoensis<br />
Nemoto <strong>and</strong> Aoki (1974)<br />
Dick, Buschman, <strong>and</strong> Ramoska<br />
(1992)<br />
Fisher (1951)<br />
Rameseshiah (1971)<br />
Oligonychus<br />
pratensis<br />
Panonychus citri<br />
Saba (1971)<br />
Smith <strong>and</strong> Furr (1975)<br />
Tetranychus ludeni<br />
Tetranychus tumidus<br />
Tetranychus urticae<br />
Neozygites<br />
tanajoae<br />
Mononychellus<br />
tanajoa<br />
Tetranychidae<br />
Delalibera, Hajek, <strong>and</strong> Humber<br />
(2004)<br />
Oligonychus gossypii<br />
Neozygites<br />
tetranychid<br />
Tarichium<br />
acaricolum<br />
Tarichium<br />
azygosporicum<br />
Tarichium<br />
distinctum<br />
Tetranychus urticae Tetranychidae Weiser (1968)<br />
Pergamasus sp. Parasitidae Bałazy <strong>and</strong> Wiśniewski (1984)<br />
Pergamasus sp. Parasitidae Bałazy, Wiśniewski, <strong>and</strong><br />
Kaczmarek (1987)<br />
Pergamasus sp. Parasitidae Bałazy et al. (1987)<br />
Tarichium<br />
hyalinum<br />
Tarichium<br />
monokaryoticum<br />
Tectocepheus<br />
velatus<br />
Tricouropoda<br />
szczecinensis<br />
Parasitidae Bałazy et al. (1987)<br />
Uropodidae Bałazy et al. (1987)
MITE PATHOGENS IN IPM<br />
267<br />
Table 2 Continued<br />
Tarichium<br />
svalbardense<br />
Dinychus carinatus<br />
Pergamasus sp.<br />
Veigaia sp.<br />
Prodinychidae<br />
Parasitidae<br />
Veigaiidae<br />
Bałazy et al. (1987)<br />
Bałazy <strong>and</strong> Wiśniewski<br />
(1984)<br />
Bałazy et al., 1987<br />
Tarichium<br />
obtusoangulatum<br />
Uropoda minima Uropodidae Bałazy <strong>and</strong> Wiśniewski<br />
(1984)<br />
Tarichium pusillum Pergamasus sp. Parasitidae Bałazy <strong>and</strong> Wiśniewski<br />
(1984)<br />
Tarichium<br />
sphaericum<br />
Trachyuropoda<br />
coccinea<br />
Trachyuropodidae<br />
Bałazy <strong>and</strong> Wiśniewski<br />
(1984)<br />
Tarichium<br />
subglobosum<br />
Pergamasus sp.<br />
Uropoda minima<br />
Parasitidae<br />
Uropodidae<br />
Bałazy <strong>and</strong> Wiśniewski<br />
(1984)<br />
Bałazy <strong>and</strong> Wiśniewski<br />
(1984)<br />
Tarichium<br />
tenuisculpturatum<br />
Pergamasus sp. Parasitidae Bałazy <strong>and</strong> Wiśniewski<br />
(1984)<br />
Tarichium<br />
uropodinis<br />
Trachyuropoda<br />
coccinea<br />
Trachyuropodidae<br />
Bałazy <strong>and</strong> Wiśniewski<br />
(1982)<br />
Tarichium<br />
verruculosum<br />
Celaenopsis sp.<br />
Unidentified<br />
Celaenopsidae<br />
Galumnidae<br />
Bałazy et al. (1987)<br />
4.1.2. Natural Entomophthoraceous Infections<br />
The first record of an entomophthoralean fungus infection in spider mites was<br />
observed <strong>by</strong> Fisher (1951) who noted adult mortality from 32 to 95% in populations<br />
of the citrus red mite Panonychus citri. The fungus was in particular prevalent<br />
during late summer <strong>and</strong> early autumn throughout the Florida peninsula. Weiser <strong>and</strong><br />
Muma (1966) isolated the fungus later from the Texas citrus mite Eutetranychus<br />
banksi <strong>and</strong> described it as Entomophthora floridana. The fungus has since been<br />
reported from several other spider mites species: For example, it was observed in<br />
Tetranychus tumidis on cotton in the humid subtropical regions of Florida (Saba,<br />
1971), in T. evansi on tomato crops in Brazil (Humber et al., 1981), in T. ludeni<br />
on bean in India (Ramaseshiah, 1971), in Oligonychus hondoensis on cedar in<br />
Japan (Nemoto & Aoki, 1975) <strong>and</strong> in T. urticae on field corn in North Carolina,<br />
USA (Br<strong>and</strong>enburg & Kennedy, 1982). The fungus has also been reported in<br />
Pol<strong>and</strong> on the twospotted spider mite T. urticae <strong>and</strong> on Bryobia sp. (Mieţkiewski<br />
et al., 1993).<br />
Keller <strong>and</strong> Wuest (1983) noted infections <strong>by</strong> Neozygites adjarica in T. urticae<br />
on bean in Switzerl<strong>and</strong>, but later investigations showed that this fungus is identical<br />
to N. floridana; N. tetranychi, described <strong>by</strong> Weiser (1968) as a pathogen of the
268<br />
L.P.S. VAN DER GEEST<br />
twospotted spider mite from a fruit orchard in Southern Bohemia, Czech Republic, is<br />
also considered to be a synonym of N. floridana (Keller, 1997).<br />
Bridge <strong>and</strong> Worl<strong>and</strong> (2008) observed a Neozygites infection in the<br />
cryprostigmatic mite Alaskozetes antarcticus (Ameronothridae). This mite was<br />
collected at Rip Point, Nelson Isl<strong>and</strong> off the West coast of the Antarctic peninsula. A<br />
few specimens appeared to be infected <strong>by</strong> a fungus that was provisionally described<br />
as Neozygites cf. acaridis. The mite survives the harsh climatic conditions <strong>by</strong><br />
lowering the freezing point <strong>by</strong> the accumulation of low molecular weight<br />
cryoprotective compounds such as glycerol, together with the removal or masking of<br />
ice-nucleating substances from its body.<br />
The introduction of the cassava green mite Mononychellus tanajoa into the<br />
cassava growing regions on the African continent has led to a comprehensive search<br />
for natural enemies of this pest. This has resulted in the isolation of a Neozygites sp.<br />
that is very specific for the cassava green mite in Venezuela <strong>by</strong> Agudela-Silva (1986)<br />
<strong>and</strong> later also in Brazil <strong>by</strong> Delalibera et al. (1992). The fungus is also known from the<br />
African continent. Originally, the fungus was considered to be identical to N.<br />
floridana, although it did show differences in, among others, its very restricted host<br />
spectrum <strong>and</strong> in the size of the conidia. Recently, the fungus has been described as N.<br />
tanajoae (Delalibera et al., 2004). It can be distinguished from N. floridana on the<br />
basis of 18S ribosomal DNA (rDNA) sequences, host range, nutritional requirement<br />
for growth in vitro, tolerances to low temperatures (4° C) <strong>and</strong> ability to withst<strong>and</strong><br />
specific cryopreservation techniques. N. tanajoae isolates from Brazil <strong>and</strong> Africa have<br />
identical 18S rDNA sequences but they presented 5.7 <strong>and</strong> 9.94% pair wise distance<br />
from N. floridana isolates. N. tanajoae proved to differ sufficiently from other mitepathogenic<br />
fungi referred to as N. floridana to justify the description as a new species.<br />
4.1.3. Role of Neozygites floridana in the Field<br />
The role of Neozygites spp. in the field has been studied in a number of instances.<br />
Numerous examples show that Neozygites sp. may have a major impact on<br />
populations of spider mites in agricultural crops. Saba (1971) observed Neozygites<br />
floridana in populations of T. tumidus in cotton field in the humid subtropical part of<br />
Florida. A reduction of 220 spider mites per cotton leaf down to less than 1 spider<br />
mite was noted during a period of warm humid weather with heavy rainfall. This<br />
reduction could be mainly attributed to the presence of the fungus disease. Similar<br />
observations were made <strong>by</strong> others, e.g. Smith <strong>and</strong> Furr (1975) who established that<br />
Neozygites in the main factor that limits late-season population increases of T.<br />
urticae on cotton in the delta of the Mississippi <strong>and</strong> Carner (1976) who found the<br />
fungus throughout the states Ge<strong>org</strong>ia, South Carolina <strong>and</strong> Alabama. He considered<br />
Neozygites a very important factor in regulating spider mite populations in cotton.<br />
Treatment of crops with fungicides may affect the incidence of fungus disease<br />
in populations of spider mite: Br<strong>and</strong>enburg <strong>and</strong> Kennedy (1983) observed a lower<br />
proportion of spider mites infected <strong>by</strong> Neozygites in lima beans when the fungicide<br />
benomyl was applied. The fungicide did not affect sporulation of the pathogen, but<br />
seemed to have an effect on conidial germination <strong>and</strong> growth of the fungus.
MITE PATHOGENS IN IPM<br />
269<br />
Immature stages of T. urticae are more susceptible to N. floridana than adult<br />
mites, while adult females are more susceptible to infection than adult males (Susilo<br />
Nordin, & Brown, 1994). The authors suggest than the thinner cuticle of the<br />
immature mites could be the cause that immature stages are more vulnerable to the<br />
fungus disease. That males are less susceptible to infection is probably due to the<br />
stronger cuticle of this sex compared to that of females. Males have to compete with<br />
other males for females which may have resulted in a tougher cuticle. On the other<br />
h<strong>and</strong>, females have a more elastic opisthosomal cuticle, needed for ovarial<br />
development <strong>and</strong> oviposition. The authors speculate that the cuticle of females might<br />
be thinner, or somewhat different in chemical composition.<br />
Infection <strong>by</strong> entomogenous fungi results from penetration of the fungus through<br />
the cuticle of the host <strong>by</strong> a combination of enzymatic <strong>and</strong> mechanical processes.<br />
Successful infection <strong>by</strong> a fungus depends largely on the effectiveness of various<br />
antifungal substances present in the host cuticle. The authors claim that differential<br />
susceptibility of different stages <strong>and</strong> sexes of mites can be attributed partially to the<br />
presence or absence of antifungal substances. This finding is in contrast with<br />
observations <strong>by</strong> Elliot (1998) on an epizootic of Neozygites tanajoae in the cassava<br />
green mite M. tanajoa in Brazil. Far fewer capilliconidia of the fungus were found<br />
on field-collected juveniles than on adult females, while the vast majority of killed<br />
mycosed mites were adult females. Elliot (1998) assumed that the limited movement<br />
of immature stages makes them less likely to pick up capilliconidia from the leaf<br />
surface. For additional information on the role of N. floridana in natural populations<br />
of spider mites is referred to Van der Geest et al. (2000).<br />
4.1.4. The Cassava Green Mite <strong>and</strong> Neozygites tanajoae<br />
The unfortunate introduction of the cassava green mite (GCM), M. tanajoa, from<br />
Latin America into East Africa during the 1970s led to a comprehensive search for<br />
natural enemies of this pest. The mite dispersed within 10 years across the cassava<br />
belt in Africa, threatening cassava production in vast areas of the continent<br />
(Yaninek, 1988). It was already clear from the beginning that chemical control of the<br />
CGM would be no option. Cassava is a marginal crop in Africa <strong>and</strong> the farmers<br />
would not be able to afford the cost of chemical control. Moreover, chemical control<br />
would result in an unacceptable environmental pollution in large parts of the<br />
continent. It was clearly understood that classical biological control would be the<br />
most desirable solution for the problem. Several predatory mites of the family<br />
Phytoseiidae were collected in various locations in Latin America <strong>and</strong> introduced<br />
into Africa.<br />
During the search for natural enemies, also a species of Neozygites was found,<br />
first in Venezuela (Agudela-Silva, 1986), later also in Brazil <strong>by</strong> Delalibera et al.<br />
(1992). The fungus has a very narrow host spectrum <strong>and</strong> does not infect other spider<br />
mites or predatory mites. The fungus, initially considered to be N. floridana, but<br />
later described <strong>by</strong> Delalibera et al., (2004) as Neozygites tanajoae, is considered a<br />
good c<strong>and</strong>idate as biological control agent for the CGM in Africa, because of its<br />
high specificity (De Moraes & Delalibera, 1992). A drawback, however, is the fact
270<br />
L.P.S. VAN DER GEEST<br />
that the fungus cannot successfully be grown on artificial media (Leite, Smith, De<br />
Moraes, & Roberts, 2000), which means that it should be released in the field in the<br />
form of fungus infected dead mites. A detailed study was therefore performed in<br />
order to gain information on the suitability of the fungus as biocontrol agent. In a<br />
series of experiments, Oduor, De Moraes, Yaninek, <strong>and</strong> Van der Geest (1995a),<br />
Oduor, Yaninek, Van der Geest, <strong>and</strong> De Moraes (1995b), Oduor (1995c), Oduor, De<br />
Moraes, Van der Geest, <strong>and</strong> Yaninek (1996a), Oduor, Yaninek, Van der Geest, <strong>and</strong><br />
De Moraes (1996b), Oduor, De Moraes, Van der Geest, <strong>and</strong> Yaninek (1997a) <strong>and</strong><br />
Oduor, Sabelis, Lingeman, De Moraes, <strong>and</strong> Yaninek (1997b) studied the biology of<br />
N. tanajoae <strong>and</strong> its effect on the CGM. They demonstrated that the production of<br />
primary conidia is affected <strong>by</strong> ambient humidity, temperature <strong>and</strong> photoperiod:<br />
production of conidia increased with higher temperatures between 13°C <strong>and</strong> 23°C,<br />
but no conidia production was obtained above 28°C. Also, germination of<br />
capilliconidia on cassava green mites is affected <strong>by</strong> exposure time, temperatures,<br />
ambient humidity <strong>and</strong> photoperiod.<br />
Infectivity of capilliconidia is lost after several days: only 3.5% of the spores<br />
germinate after a storage period of 10 days. It was also found that germination<br />
occurred at all temperatures studied (13–33°C), even at 13°C, more than 15% of the<br />
capilliconidia germinated. This is an indication that the minimum temperature for<br />
germination may still be lower. An interesting observation is also that more<br />
capilliconidia germinate at 18°C than at higher temperatures. Germination in the<br />
dark is considerably higher than in light, while this process is also greatly affected<br />
<strong>by</strong> ambient humidity. The fungus apparently sporulates under natural conditions<br />
early in the morning before sunrise when the temperature is still low <strong>and</strong> the relative<br />
humidity high. Primary conidia can then disperse <strong>and</strong> produce capilliconidia that<br />
wait on the leaf surface to be picked up <strong>by</strong> a suitable host.<br />
N. tanajoae cannot be mass produced in artificial culture media. Propagation<br />
needs to be performed in live mites, which is a laborious, <strong>and</strong> also expensive<br />
process. Storage of dead, non-sporulating infected mites (also called mummies)<br />
appears to be possible over prolonged periods of time in well-sealed plastic<br />
containers with cotton wool partially soaked in glycerol to establish a low humidity.<br />
In this manner, the fungus remains viable for periods of 6–7 months.<br />
The fungus causes significant reductions in cassava green mite populations in<br />
cassava fields in the State of Bahia, Brazil (Delalibera, De Moraes, & Sosa Gomez,<br />
1999), reaching infection levels up to 75% during the wet season. Elliot et al. (2000)<br />
conducted a 4-year study in cassava fields in a semi-arid region in northeastern<br />
Brazil. The authors found that the fungus had a significant effect on CGM<br />
populations, but results were not very consistent for the different years. The fungus<br />
was not found in live mites during dry periods <strong>and</strong> for that reason it was assumed<br />
that resting spores were the most feasible mechanism to survive these periods of<br />
drought. Resting spores were found in great numbers during an epizootic in 1995, but<br />
they were not found in epizootics in early <strong>and</strong> mid 1998. Elliot (1998) considered<br />
perennial survival in the field of the fungus in mummies highly improbable as<br />
experiments had demonstrated that no viable fungus could be detected in dead mites<br />
after 2 month of hot <strong>and</strong> dry storage, both in the field <strong>and</strong> in the laboratory. In a later<br />
report, Elliot, De Moraes <strong>and</strong> Mumford (2008) discussed results of an experiment in
MITE PATHOGENS IN IPM<br />
271<br />
which they monitored a population of the CGM <strong>and</strong> its natural enemies in central<br />
Bahia. Despite the presence of very high levels of the predatory mite Neoseiulus<br />
idaeus, there was an overexploitation of the cassava plants <strong>by</strong> the cassava green<br />
mite, which led to a total leaf loss. A simple regression model predicted a potential<br />
epizootic <strong>by</strong> N. tanajoae, but at that time, no inoculum of the fungus was present.<br />
There could have been an epizootic after the CGM population crashed, but then<br />
there were no hosts present to infect. The study showed the ineffectiveness of the<br />
predator <strong>and</strong> the importance of a correct timing of the pathogen. The authors<br />
concluded that the fungus may be a useful addition to biological control in this<br />
system with another predator than N. idaeus.<br />
Yaninek et al. (1996) carried out a survey of fungi occurring in mites in the<br />
Republic of Benin, West Africa <strong>and</strong> found N. tanajoae in CGM <strong>and</strong> in<br />
Oligonychus gossypii. The fungus was present during the entire year, although<br />
the incidence of the disease was considerably greater in the wet season.<br />
Infection levels reached <strong>by</strong> the Benin strain were never as high as those of the<br />
Brazilian isolates where infection levels close to 100% may sometimes be<br />
reached. However, disease incidences in O. gossypii were about twice as high as<br />
in CGM. This species of mite is indigenous to Africa, in contrast to the cassava<br />
green mite. The N. tanajoae strains native to Africa are thought to be weakly<br />
pathogenic towards the CGM as they cause only low levels of mortality in CGM<br />
populations.<br />
Based on these studies, N. tanajoae pathotypes from Latin America were<br />
being considered as a biological control agent of the CGM in Africa. An<br />
international collaboration between the International Institute for Tropical<br />
Agriculture (IITA, Cotonou, Benin), Empresa Brasileira de Pesquisa<br />
Agropecuária (EMBRAPA, Brazil) <strong>and</strong> the University of Amsterdam (The<br />
Netherl<strong>and</strong>s) was set up in order to guide the introduction <strong>and</strong> release of the<br />
fungus into Africa. An in vivo release procedure has been developed at the<br />
(IITA) as it is not yet possible to culture the fungus in artificial culture media.<br />
Field experimental releases were performed in order to test the possibility to<br />
induce the development of epizootics in the field (Hountondji, 2005). The in<br />
vivo release method consisted of the release of 1-day old infected mites on<br />
young leaves of with CGM infested cassava fields Two different Brazilian<br />
strains were released in Southeastern Benin, resulting in disease incidence levels<br />
of 34 <strong>and</strong> 26.5% respectively, while the maximum prevalence for a Beninese<br />
isolate was only 4.5%. The fungus is in the first site endemically present, but<br />
had never been found in northeastern Benin. Post-release monitoring in<br />
Southeastern Benin showed after 10 months the presence of the fungus in 3 out<br />
of 20 cassava field where the fungus had been released. In Northeastern Benin,<br />
epizootics were also observed with infection levels between 15 <strong>and</strong> 70%. An<br />
interesting observation is that infection levels were consistently higher in fields<br />
inoculated with Brazilian isolates compared to those inoculated with the<br />
Beninese isolates.<br />
The epizootics were especially observed during periods of hot days <strong>and</strong> cool<br />
nights with high relative humidity. The establishment of the Brazilian isolates at the<br />
release site could be confirmed. However, resting spores, believed to be essential for
272<br />
L.P.S. VAN DER GEEST<br />
the survival of the fungus during dry periods were hardly found. Further studies will<br />
be needed to determine the suitability of the fungus as biocontrol agent of the CGM<br />
in Africa.<br />
Hountondji (2008) discussed the interactions within the cassava green mite-<br />
Neozygites tanajoae system. He states that most fungal pathogens lack the<br />
capacity to search for their hosts but that they have rather developed a sit-<strong>and</strong>-wait<br />
strategy. Field applications of N. tanajoae against the CRM has resulted in only<br />
limited success <strong>and</strong> for that reason, studies were conducted on the tritrophic<br />
interactions in the system. An interesting finding is that herbivores trigger the<br />
release of volatile chemicals (HIPV) that promotes sporulation of the fungal<br />
pathogen, whereas the host mites avoid the haloes of conidia. However, the mite<br />
does not avoid the pathogen when the fungus is inside the mummified cadaver.<br />
Mechanically damaged leaves produce also volatile, but these “green leaf<br />
volatiles” seem to delay sporulation. Hountondji (2005) speculates that a delay in<br />
the formation of conidia until the HIPV’s are produced is to the advantage of the<br />
fungus. The production of HIPV’s is a signal for the fungus that herbivores (hosts<br />
for the fungus) are present.<br />
4.2. Deuteromycetes<br />
The Deuteromycetes, also mitosporic or anamorphic fungi, <strong>and</strong> formerly called the<br />
Fungi Imperfecti, is a group of fungi of which no sexual stage is known. It is<br />
difficult to place these fungi in the fungus classification system, since this<br />
classification is mainly based on the mode of sexual reproduction. The majority of<br />
Deuteromycetes are probably the asexual stages of Ascomycota <strong>and</strong> Basidiomycota,<br />
with the largest number belonging to the Ascomycota. The approximately 20,000<br />
species (2,600 genera) of Deuteromycetes (or Deuteromycota) lack any common<br />
phylogenetic origin or relationship <strong>and</strong> have only been grouped together for the sake<br />
of convenience. Classification of Deuteromycetes is mainly based on morphological<br />
similarities. The criteria typically used are color, shape, size <strong>and</strong> septation of the<br />
conidia (whether the spores are unicellular, or made up of multiple cells). The effect<br />
of this classification is that unrelated fungi have been “lumped” together while<br />
possibly related fungi have been classified into different form-classes because of<br />
differences in the visual appearance of the spores. When the sexual stage<br />
(teleomorph) is discovered, the correct name of the fungus will be that of the<br />
teleomorph.<br />
A group in the Deuteromycetes is the form-class Hyphomycetes. These fungi<br />
have a mycelium but lack a sporocarp (structure in which spores are formed). The<br />
spores are borne on separate or aggregated conidiophores (stroma). We speak of a<br />
synnema when the conidiophores are united at the base <strong>and</strong> of a sporodochium when<br />
the hyphae are aggregated to a cushion-line structure on which the conidiophores are<br />
formed. Many of the spores of the Deuteromycetes have morphologically distinct<br />
features so that the spores of this group are some of the most easily identified. These<br />
fungi are also easily cultured so that more research has been conducted on this group<br />
of fungi than on many others.
MITE PATHOGENS IN IPM<br />
273<br />
4.2.1. Hirsutella Infections in Mites<br />
A well-known genus in the Hyphomycetes is Hirsutella. Approximately 80 species<br />
have been described in this genus; most species are pathogenic to tropical<br />
invertebrates, some are pathogens of Acari, in particular of eriophyids. Teleomorphs<br />
of Hirsutella have been reported as Cordyceps <strong>and</strong> Torrubiella spp. (cf. Ch<strong>and</strong>ler<br />
et al., 2000). Hirsutella species observed in mites are given in Table 3.<br />
The first published report of a Hirsutella infection in an eriophyid goes back to<br />
1924: Speare <strong>and</strong> Yothers (1924) observed a sudden decimation of a large<br />
population of the citrus red mite (CRM) (Phyllocoptruta oleivora) on grapefruit in<br />
Florida. The population density of CRM was in June sometimes extremely high with<br />
5,000 mites on a single grapefruit, but soon after the maximum density had been<br />
reached, populations went down to almost zero. The authors were able to discern<br />
fungal hyphae in mite cadavers <strong>and</strong> also noted that disease incidence was much<br />
lower after application of a fungicidal copper spray. Fisher (1950) described this<br />
fungus later as Hirsutella thompsonii (Fig. 3).<br />
Figure 3. Epitremerus goniathrix (Eriophyidae), infected <strong>by</strong> Hirsutella sp.<br />
Photograph: Leo P.S. van der Geest.<br />
The conidia are the infective propagules of the fungus. They are formed on<br />
phialides (flask-like conidiophores) that taper into a long narrow neck, <strong>and</strong> produce<br />
usually only 1–3 conidia in a dense terminal sphere of slime. This gives the<br />
impression that only one spore on each phialide is produced (Fig. 4). The mucous<br />
coat facilitates adhesion of the spores to the host cuticle. Penetration of the fungus is<br />
usually through all parts of the host’s body, but in case of spider mites, it is usually<br />
through the legs. The fungi enter the host through the cuticle which is composed of<br />
about 30% chitin embedded in a protein matrix. Entomogenous fungi often produce<br />
proteases that may play a role in the early stages of penetration <strong>by</strong> exposing the<br />
chitin fibrils. Subsequently, chitinolytic enzymes are excreted that causes<br />
degradation of the fibrils into chains of glucose-N-acetyl of variable length.
274<br />
L.P.S. VAN DER GEEST<br />
Table 3. Hirsutella species infecting mites <strong>and</strong> their hosts.<br />
Fungus species Mite species Mite family Reference<br />
Hirsutella sp.<br />
Amrineus cocofolius<br />
Epitremerus goniathrix<br />
Eriophyoidea Van der Geest et al. (2002)<br />
Mononychellus sp.<br />
Notostrix attenuata<br />
Tetranychidae<br />
Eriophyoidea<br />
Bartkowski et al. (1988)<br />
Van der Geest et al. (2002)<br />
Pronematus sp. Tydeidae Cabrera <strong>and</strong> McCoy (1984)<br />
Propilus syagris<br />
Retracus jonhstoni<br />
Eriophyoidea Van der Geest et al. (2002)<br />
Tarsonemus sp. Tarsonemidae Van der Geest et al. (2002)<br />
H. brownorum Mites in soil Humber (1992)<br />
H. gregis Abacarus hystrix Eriophyoidea Minter, Brady, <strong>and</strong> Hall<br />
(1983)<br />
Unidentified sp. Acaridae Miętkiewski, Bałazy,<br />
<strong>and</strong><br />
Tkaczuk (2000)<br />
H. danubiensis Tetranychus urticae Tetranychidae Bałazy et al. (2008)<br />
H. haptospora Uropodina sp. Uropodoidea Humber (1992)<br />
Urobovella sp. Uropodoidea Miętkiewski et al. (2000)<br />
Unidentified species Parasitiformes Miętkiewski et al. (2000)<br />
H. kirchneri Abacarus hystrix Eriophyoidea Minter et al. (1983)<br />
Eutetranychus<br />
orientalis<br />
Tetranychidae<br />
Sztejnberg, Doron-Shloush,<br />
<strong>and</strong> Gerson (1997)<br />
Hemisarcoptes<br />
coccophagus<br />
Hemisarcoptidae Sztejnberg et al. (1997)<br />
Panonychus citri Tetranychidae Sztejnberg et al. (1997)<br />
Phyllocoptruta oleivora Eriophyoidea Cabrera <strong>and</strong> Dominguez<br />
(1987a) <strong>and</strong> Sztejnberg<br />
et al. (1997)<br />
H. necatrix Abacarus hystrix Eriophyoidea Minter et al. (1983)<br />
Tetranychus<br />
cinnabarinus<br />
Tetranychidae Sztejnberg et al. (1997)
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275<br />
Table 3 continued<br />
Dendrolaelaps cornutus Digamasellidae Miętkiewski et al. (2000)<br />
H. nodulosa Aceria guerreronis Eriophyoidea Cabrera <strong>and</strong> Dominguez<br />
(1987b)<br />
Phyllocoptruta oleivora Eriophyoidea Cabrera <strong>and</strong> Dominguez<br />
(1987a)<br />
Polyphagotarsonemus<br />
latus<br />
Tarsonemidae<br />
Peña, Osborne, <strong>and</strong> Duncan<br />
(1996)<br />
Steneotarsonemus<br />
fragariae =<br />
Phytonemus pallidus<br />
Tarsonemidae Miętkiewski et al. (2000)<br />
H. rostrata Dendrolaelaps<br />
tetraspinosus<br />
Digamasellidae<br />
Bałazy <strong>and</strong> Wiśniewski<br />
(1989)<br />
Proctolaelaps sp. Ascidae Bałazy <strong>and</strong> Wiśniewski<br />
(1989)<br />
H. thompsonii Abacarus hystrix Eriophyoidea Lewis, Heard, Brady, <strong>and</strong><br />
Minter (1981)<br />
Acalitus vaccinii Eriophyoidea Baker <strong>and</strong> Neunzig (1968)<br />
Aceria cynodoniensis Eriophyoidea McCoy (1996)<br />
Aceria guerreronis Eriophyoidea Humber (1992)<br />
Aceria sheldonii Eriophyoidea McCoy (1996) <strong>and</strong> Sosa<br />
Gomez <strong>and</strong> Moscardi (1991)<br />
Aceria sp. Eriophyoidea McCoy <strong>and</strong> Selhime (1977)<br />
Aculops lycopersici Eriophyoidea In: Ch<strong>and</strong>ler et al. (2000)<br />
Calacarus heveae Eriophyoidea Tanzini, Alves, Tamai, De<br />
Moraes, <strong>and</strong> Ferla (2000)<br />
Colomerus<br />
novahebridensis<br />
Eriophyoidea<br />
Hall, Hussey, <strong>and</strong> Mariau<br />
(1980)<br />
Epitremerus goniathrix Eriophyoidea Van der Geest et al. (2002)<br />
Notostrix formosae Eriophyoidea Van der Geest et al. (2002)<br />
Phyllocoptruta oleivora Eriophyoidea Fisher (1950)<br />
Retracus elaeis Eriophyoidea Urueta (1980)<br />
Rhynacus sp. Eriophyoidea Cabrera, Caceras, <strong>and</strong><br />
Dominguez (1987)<br />
Vasates destructor Eriophyoidea McCoy (1996)
276<br />
L.P.S. VAN DER GEEST<br />
Table 3 Continued<br />
Polyphagotarsonemus<br />
latus<br />
Tarsonemidae Peña et al. (1996)<br />
Vasates mckenzie Tarsonemidae Miętkiewski et al. (2000)<br />
Dolichotetranychus<br />
floridanus<br />
Tenuipalpidae Humber (1992)<br />
Eutetranychus banksi Tetranychidae McCoy <strong>and</strong> Selhime (1977)<br />
Eotetranychus<br />
sexmaculatus<br />
Tetranychidae McCoy <strong>and</strong> Selhime (1977)<br />
Eutetranychus<br />
orientalis<br />
Tetranychidae<br />
Gerson, Kenneth, <strong>and</strong><br />
Muttath (1979)<br />
Mononychellus tanajoa Tetranychidae Yaninek et al. (1996)<br />
Panonychus citri Tetranychidae McCoy <strong>and</strong> Selhime (1977)<br />
Oligonychus gossypii Tetranychidae Yaninek et al. (1996)<br />
Tetranychus<br />
cinnabarinus<br />
Tetranychidae<br />
Cehrnin, Gafni, Mozes-<br />
Koch, Gerson, <strong>and</strong><br />
Sztejnberg (1997)<br />
Oligonychus ilicis Tetranychidae Gardner, Oetting, <strong>and</strong><br />
Storey (1982)<br />
Tetranychus urticae Tetranychidae Gardner et al. (1982)<br />
Tetranychus turkestani Tetranychidae In: Ch<strong>and</strong>ler et al. (2000)<br />
Trachyuropoda<br />
coccinea<br />
Trachyuropodidae Bałazy <strong>and</strong> Wiśniewski<br />
(1982)<br />
H. tydeicola Lorryia formosa Tydeidae Cabrera, see: Samson <strong>and</strong><br />
McCoy (1982)<br />
Tydeus californicus Tydeidae Cabrera, see: Samson <strong>and</strong><br />
McCoy (1982)<br />
Tydeus gloveri Tydeidae Samson <strong>and</strong> McCoy (1982)<br />
H. v<strong>and</strong>ergeesti Amblyseius sp.<br />
Neoseiulus sp.<br />
Seiulus sp.<br />
Typhlodromus sp.<br />
Tarsonemus lacustris<br />
Phytoseiidae<br />
Tarsonemidae<br />
Bałazy et al. (2008)
MITE PATHOGENS IN IPM<br />
277<br />
When grown in artificial cultures, a toxic protein is produced with a molecular<br />
weight of 15–16 kDa (Vey, Quiot, Mazet, & McCoy, 1993). This protein, hirsutellin<br />
A (HtA) is a heat stable, non-glycosylated protein with properties similar to<br />
ribosome-inhibiting proteins. It is a single chain polypeptide that is composed of 130<br />
amino acids (Herrero-Galán et al., 2008). HtA shows ribotoxin activity <strong>and</strong> interacts<br />
with phospholipid membranes. When administered orally or <strong>by</strong> injection, it causes<br />
strong cytotoxic effects against several insect species (pycnosis of the nucleus <strong>and</strong><br />
lesions in the midgut, malpighian tubules, hypodermis, fatbody, hemocytes, muscles<br />
<strong>and</strong> silk gl<strong>and</strong>s of larvae). The toxin affects a wide range of arthropods, including<br />
mites. It was tested against the citrus rust mite Phyllocoptruta oleivora, the natural<br />
host of the fungus, where it caused considerable mortality among adult mites, while<br />
oviposition of females was lowered prior to their death (Omoto & McCoy, 1998).<br />
Maimala, Tarter, Bouciar, <strong>and</strong> Ch<strong>and</strong>rapatya (2002) studied 162 strains of H.<br />
thompsonii <strong>and</strong> found that more than half of these strains produced the toxin. They<br />
were able to characterize the gene encoding for the toxin, but the presence of the<br />
gene could not be associated with enhanced insecticidal properties of the fungus.<br />
Other toxins have also been reported to be produced <strong>by</strong> Hirsutella sp., such as<br />
hirsutellin B <strong>and</strong> phomalactone. It is not within the scope of this manuscript to<br />
discuss these products further.<br />
H. thompsonii regularly causes epizootics in populations of P. oleivora under natural<br />
conditions in Florida <strong>and</strong> affects both nymph <strong>and</strong> adult stages. The asexual spores are<br />
produced outside the host body on the plant surface. Conidia germinate under favorable<br />
conditions (high relative humidity) <strong>and</strong> enter the body <strong>by</strong> means of a germ tube. After<br />
penetration, a ramifying growth of the fungus can be discerned. The fungus erupts after<br />
Figure 4. Phialid of Hirsutella thompsonii with conidia. The globular structure on<br />
top of the phialid may hold several conidia which are contained in a slimy sheath.<br />
Photograph courtesy of Dr. Marcel R. Tanzini.
278<br />
L.P.S. VAN DER GEEST<br />
death of the mite through the cuticle <strong>and</strong> forms new spores. It takes about 4 h for a spore to<br />
penetrate the cuticle of the host, while time from infection to formation of new spores is<br />
around 4 days at 25–30°C (Fig. 4).<br />
The fungus can easily be grown on artificial media <strong>and</strong> this property together with its<br />
high infective potential towards the citrus rust mite (CRM) has led to research aimed at the<br />
development of the fungus as biological control agent. Large-scale laboratory <strong>and</strong> industrial<br />
production methods have been developed for the production of mycelial <strong>and</strong> conidial<br />
preparations (McCoy, Hills, & Kanavel, 1975; McCoy, 1981). It was planned to introduce<br />
the fungus early in the season as a prophylactic to reduce outbreaks of the CRM.<br />
Commercial production of conidial preparation in the USA was developed in 1975–1976<br />
<strong>by</strong> Abbott Laboratories <strong>and</strong> full registration was received for a mycoacaricide for the<br />
control of eriophyids on citrus under the name Mycar TM . Several hundreds of kilograms<br />
were sold of the product but commercial production was discontinued in 1985 as too many<br />
factors affected the stability <strong>and</strong> reliability of the acaricide.<br />
Interest in the production of H. thompsonii based acaricides for use against eriophyids<br />
continued in other countries even after the production of Mycar TM in the USA was<br />
discontinued. Experiments have been conducted in several countries, e.g. Brazil, Argentina,<br />
Mexico <strong>and</strong> Sri Lanka, but these studies have yet not led to a commercial biological control<br />
product. More successful were studies in India where the coconut mite, Aceria (Eriophyes)<br />
guerreronis, is a major constraint to coconut farming in India, the third largest producer of<br />
coconuts in the world. Biological control has been considered for a long time, despite the<br />
availability of other control methods, including chemical <strong>and</strong> botanical pesticides <strong>and</strong><br />
nutrition-based cultural methods (Sreerama Kumar & Singh, 2001; Sreerama Kumar,<br />
2006). Research has resulted in the identification of the most infective mite pathogen,<br />
H. thompsonii, as important regulator of the coconut mite (Fig. 5). Further research had led<br />
to the production of a biological acaricide, Mycohit TM , with a mixture of mycelium<br />
Figure 5. Aceria (Eriophyes) guerreronis infected <strong>by</strong> Hirsutella thompsonii.<br />
Photograph courtesy of Dr. P. Sreerama Kumar.
MITE PATHOGENS IN IPM<br />
279<br />
<strong>and</strong> conidia as active ingredients. In a series of field experiments, it was shown that<br />
Mycohit TM is a very effective acaricide that brings down the population to over 90%. For<br />
the application of the product, youngsters are hired that climb into the trees in order to<br />
carry out the applications (Figs. 6 <strong>and</strong> 7).<br />
Further research has led to the development of Mycohit-M TM , a preparation that<br />
contains only mycelium (Sreerama Kumar & Singh, 2008). The authors also studied<br />
the effect of several adjuvants (glycerol, yeast extract powder <strong>and</strong> dehydrated malt<br />
extract) on the growth <strong>and</strong> spore forming of the latter preparation. In the presence of<br />
these adjuvants H. thompsonii biomass produced under laboratory conditions more<br />
colonies <strong>and</strong> a higher number of conidia. These products also showed protection<br />
against sun irradiation under field conditions. Studies are presently also conducted in<br />
Brazil on the control of the coconut mite <strong>by</strong> use of H. thompsonii (cf. Van der Geest<br />
et. al., 2000). Various isolates of the fungus were introduced from Mexico into Brazil<br />
<strong>and</strong> were mass produced on rice <strong>and</strong> corn grids, but the mortality due to the fungus was<br />
too low (about 35%). However, it was possible to increase the virulence of the fungus <strong>by</strong><br />
passage through the host. The fungus has been established in the field, although damage<br />
due to A. guerreronis is still too high.<br />
Figure 6. Spraying of coconut trees with Mycohit. Photograph courtesy of<br />
Dr. P. Sreerama Kumar.
280<br />
L.P.S. VAN DER GEEST<br />
Several attempts have been made to use the fungus also for the control of other<br />
mite pests. However, most of these attempts were unsuccessful, as e.g. the control of<br />
spider mites (T. cinnabarinus, Eotetranychus orientalis <strong>and</strong> T. urticae in<br />
greenhouses (Rombach & Gillespie, 1988). Hirsutella kirchneri has also been<br />
considered a good c<strong>and</strong>idate for the control of plant-inhabiting mites. Its<br />
pathogenicity was tested <strong>by</strong> Sztejnberg et al. (1997) against a number of different<br />
mites. It was shown to be effective against the eriophyid P. oleivora, <strong>and</strong> against the<br />
spider mites Eutetranychus orientalis, Panonychus citri, T. cinnabarinus <strong>and</strong> in<br />
some degree against Hemisarcoptes coccophagus (Hemisarcoptidae). However, no<br />
infectivity was found towards the broad mite Polyphagotarsonemus latus<br />
(Tarsonemidae), Rhizoglyphus robini, Tyrophagus putrescentiae (Acaridae) <strong>and</strong><br />
Typhlodromus athiasae (Phytoseiidae). No infectivity was noted towards a number<br />
of beneficial arthropods.<br />
Figure 7. Spraying of coconut trees with Mycohit. Photograph courtesy<br />
of Dr. P. Sreerama Kumar.<br />
A few reports deal with the occurrence of the H. thompsonii on the cassava<br />
green mite M. tanajoa in the cassava belt in Africa. Yaninek et al. (1996) observed
MITE PATHOGENS IN IPM<br />
281<br />
the fungus on CGM <strong>and</strong> on Oligonychus gossypii during an inventory in Benin, <strong>and</strong><br />
Odongo, Odindo, Brownbridge, <strong>and</strong> Kumar (1998) carried out experiments in which<br />
CGM infected plants were treated with suspensions of H. thompsonii. In the treated<br />
plots, 76.6% disease incidence was obtained, but rainfall caused a reduction in<br />
disease prevalence in the mites. The authors concluded that the application of the<br />
fungus has promise for controlling the CGM, but that the fungus should be applied<br />
in harmony with other natural mortality factors such as rainfall.<br />
The fungus has also been recorded in Calacarus heveae (Eriophyidae) an<br />
important pest in rubber plantations in Brazil (Tanzini et al., 2000). This mite is a<br />
major pest in the Michelin rubber plantation in Itiquira, Mato Grosso, where it<br />
causes considerable economic damage. Calacarus heveae feeds on the upper side of<br />
the leaves, in contract to most other rust mites (Figs. 8 <strong>and</strong> 9). Populations of several<br />
hundreds of mites per rubber tree leave are no exception. However, the mite<br />
populations are usually decimated after a few weeks <strong>by</strong> the action of Hirsutella<br />
thompsonii (Figs. 9 <strong>and</strong> 10). These epidemics are usually too late to avoid damage to<br />
the plantation (defoliation of the trees).<br />
Figure 8. Calacarus heveae, killed <strong>by</strong> Hirsutella thompsonii. Photograph:<br />
Leo P.S. van der Geest.<br />
Hirsutella thompsonii is normally associated with prostigmatic mites<br />
(Eriophyidae <strong>and</strong> Tetranychidae), although it has also been observed to infect<br />
mesostigmatic mites (McCoy & Selhime, 1977; Bałazy & Wiśniewski, 1982).<br />
Gerson, Gafni, Paz, <strong>and</strong> Sztejnberg (2008) tested Hirsutella thompsonii, H.<br />
kirchneri <strong>and</strong> H. necatrix with respect to their effect on several mite species: spider<br />
mites, rust mites, broad mites, but also scavengers <strong>and</strong> predatory mites were<br />
included in the study. The results of these experiments led to the conclusion that<br />
none of these fungus species gave satisfactory control of mite pests, neither in<br />
greenhouses, nor outdoors.
282<br />
L.P.S. VAN DER GEEST<br />
Figure 9. Rubber tree leaves with numerous cadavers of Calacarus heveae. The<br />
mites have been killed <strong>by</strong> the fungus Hirsutella thompsonii. However, the<br />
disease cannot prevent substantial economic damage to the rubber<br />
plantations in Itiquira, MG, Brazil, as the epidemics come too late in the<br />
season. Photograph courtesy of Dr. Marcel R. Tanzini.<br />
Figure 10. Calacarus heveae (Eriophyidae), killed <strong>by</strong> Hirsutella thompsonii. Photograph<br />
courtesy of Dr. Marcel R. Tanzini.<br />
4.2.2. Other Deuteromycetes Infecting Mites<br />
Some of the other Deuteromycetes are probably the most comprehensively studied<br />
entomopathogenic fungi. However, of these fungi, only few records have been made<br />
of natural infections in mites. Leatherdale (1965) observed a mycosis of the<br />
blackcurrant mite Cecidophyopsis ribis <strong>by</strong> Paecilomyces eriophytis, later also found
MITE PATHOGENS IN IPM<br />
283<br />
in <strong>Italy</strong> on Phytoptus avellanae, a mite causing big bud disease in ornamental <strong>and</strong><br />
fruiting hazel (Corylus avellana). Experiments were carried out with the fungus<br />
isolate from C. ribis to infect the European red mite Panonychus ulmi <strong>and</strong> the<br />
eriophyids Aceria hippocastani (from horse chestnut) <strong>and</strong> Cecidophyes galii (from<br />
goosegrass). The fungus proved to be pathogenic for the first two species, but no<br />
infection was obtained in C. galii. The fungus has also been reported <strong>by</strong> Baker <strong>and</strong><br />
Neunzig (1968): high infection rates were noted in the blueberry bud mite Aceria<br />
vaccinii (Eriophyidae) in North Carolina, USA, when high temperatures coincided<br />
with heavy rainfall <strong>and</strong> high relative humidity. Disease incidence declined from<br />
August onwards, when conditions were less favorable for the fungus. The population<br />
density of the blueberry mites then increased.<br />
One of the earliest experiments in which a fungus was tested against a<br />
phytophagous mite was a field application of B. bassiana spores for the control of<br />
the twospotted spider mite T. urticae (Dresner, 1949). Mites were treated with a dust<br />
containing 0.5% spores of the fungus, resulting in a mortality of 71%. However,<br />
these experiments did not lead to the development of a microbial acaricide.<br />
Deuteromycetes have widely been studied for the control of insect (<strong>and</strong> in a few<br />
instances mite) pests. A number of these fungi (e.g. Metarhizium, Beauveria) have a<br />
broad host spectrum <strong>and</strong> can easily be mass produced on relatively simple culture<br />
media. In Brazil, research is being conducted to evaluate several Deuteromycetes as<br />
possible control agent of the twospotted spider mite (Tamai, Alves, Lopes & Neves<br />
1998). They tested 152 different isolates for the fungi B. bassiana, B. brongniartii,<br />
Beauveria sp., Metarhizium sp., Paecilomyces lilacinus <strong>and</strong> P. farinosus. Only<br />
isolates of Beauveria spp. caused mortality between 35 <strong>and</strong> 95%. The pathogenicity<br />
of some isolates was further tested: one isolate gave even better control than<br />
obtained with chemical pesticides. The fungus was also effective against other pests<br />
in chrysanthemum, such as thrips <strong>and</strong> aphids (Alves, Tamai, & Lopes, 1998).<br />
Three different fungus species were investigated <strong>by</strong> Peña et al. (1996) with<br />
respect to their potential as biological control agent of the broad mite<br />
Polyphagotarsonemus latus (Tarsonemidae). This very polyphagous pest species<br />
thrives under warm <strong>and</strong> humid conditions, <strong>and</strong> this seemed to be a good reason to<br />
study the feasibility of using fungi as control agents. Three fungi were tested: B.<br />
bassiana, H. thompsonii <strong>and</strong> Paecilomyces fumosoroseus under controlled<br />
temperature <strong>and</strong> humidity conditions in the laboratory <strong>and</strong> in the greenhouse. All<br />
fungi were capable to infect the mites: higher doses resulted in a faster death of the<br />
mites, while density of the mites also affected disease incidence. The authors<br />
concluded from their experiments that the fungus selected should cause epizootics<br />
within 2–3 days following application. Promising results for the control of the broad<br />
mite on mulberry have been obtained with M. anisopliae <strong>by</strong> Maketon, Orosz-<br />
Coghlan, <strong>and</strong> Sinprasert (2008). The fungus is effective against larvae <strong>and</strong> adults,<br />
but no ovicidal effect was noted. The broad mite has also been found in association<br />
with Hirsutella nodulosa (Peña et al., 1996). No other associations of this mite with<br />
fungi have been reported.<br />
Shi, Feng, <strong>and</strong> Liu (2008) noted an ovicidal effect of sprays of an emulsifiable<br />
B. bassiana formulation against the twospotted spider mite T. urticae. The fungal<br />
isolate was obtained from mycosed aphids <strong>and</strong> has been formulated for the control
284<br />
L.P.S. VAN DER GEEST<br />
of whiteflies in greenhouses. The dried conidial powder was suspended in a mixture<br />
of 95% industrial paraffin as oil carrier <strong>and</strong> 5% fatty alcohol polyethylene glycol<br />
ether as emulsifier. The authors are of the opinion that the formulation has greatly<br />
enhanced egg mortality, also at lower relative humidities. Oily formulations may<br />
give a better attachment of the conidia to the target pest <strong>and</strong> a better protection of the<br />
conidia against desiccation. The formulation has also provided significant control of<br />
the citrus rust mite in orchards in East China <strong>and</strong> of T. truncates <strong>and</strong> T. turkestani in<br />
cotton in the Tarim Basin of northwest China.<br />
Isolates of fungi may show large differences in virulence to their hosts. For<br />
example, Bugeme, Maniania, Knapp, <strong>and</strong> Boga (2008) studied 23 isolates of<br />
Metarhizium anisopliae <strong>and</strong> 3 isolates of B. bassiana with respect to their<br />
pathogenicity versus the spider mite T. evansi. Temperature greatly affected<br />
observed mortality of the spider mites, but also germination of the spores <strong>and</strong><br />
growth were affected <strong>and</strong> varied with isolate.<br />
The fungi M. anisopliae <strong>and</strong> H. thompsonii are being investigated as control<br />
agents of Varroa jacobsoni (Kanga, James, & Boucias, 2002). They are pathogenic<br />
for the varroa mite <strong>and</strong> the conditions under which they can infect mites are similar<br />
to those found in bee colonies. Meikle, Mercadier, Holst, <strong>and</strong> Girod (2008) studied<br />
the impact of formulations of B. bassiana on varroa mites <strong>and</strong> on the honey bees.<br />
They formulated conidial preparations of two strains of the fungus with either<br />
carnauba or c<strong>and</strong>elilla wax powder <strong>and</strong> studied the effect on colony health <strong>and</strong> mite<br />
fall (mortality). Bees were nof affected <strong>by</strong> the fungal preparations, but mite fall was<br />
consistently higher than the control. Results were encouraging, but more knowledge<br />
should be acquired on conidia dosage, number of applications <strong>and</strong> conditions within<br />
the bee hives.<br />
Eken <strong>and</strong> Hayat (2008) conducted an inventory for natural enemies of the<br />
twospotted spider mite Tetranychus urticae in Turkey. They found several isolates<br />
of Cladosporium cladosporioides (Moniliaceae), that were subsequently tested in<br />
the laboratory with respect to their pathogenicity towards T. urticae. The fungus<br />
caused mortality levels of 51–75% when sprayed on leaflets infested with<br />
twospotted spider mites. These results are encouraging <strong>and</strong> additional experiments<br />
should be conducted. Cladosporium infections were also found <strong>by</strong> Van der Geest et<br />
al. (2002) in Retracus johnstoni, an eriophyid feeding on the palm tree Syagrus<br />
romanzoffiana in Brazil. The fungus has been isolated on potato-dextrose agar, but<br />
no further experiments have been carried out with this isolate.<br />
Interesting experiments were performed <strong>by</strong> Sanassi <strong>and</strong> Amirthavalli (1970)<br />
with the velvet mite Trombidium gigas (Trombidiidae). Mite were infected with<br />
spores of the fungus Aspergillus flavus, a fungus also capable of infecting humans<br />
<strong>and</strong> problematic in foods as it produces the very toxic aflatoxin. Three different<br />
methods were applied: injection of spore suspensions into the body cavity, spraying<br />
of spore’s suspensions on the integument of the mite <strong>and</strong> dusting of spores on the<br />
integument. In all cases infection of the mites was obtained. Changes in the structure<br />
of the integument were noted (Sanassi & Oliver, 1971). The first sign of the disease<br />
is the loss of the scarlet-red plumose cuticular setae of the mites. Each seta consists<br />
of a main central stem from where minor secondary branches arise. The base of the
MITE PATHOGENS IN IPM<br />
285<br />
central stem is normally slightly enlarged <strong>and</strong> is buried in sockets present in the epi<strong>and</strong><br />
procuticle.<br />
The fungus apparently digests the lipoproteinaceous epicuticular layer that<br />
attaches the base to the cuticular sockets. Subsequently, the process is followed <strong>by</strong><br />
additional chemical changes in the composition of the cuticle. Epidermal cells<br />
display interesting pathological symptoms. In uninfected mites, epidermal cells form<br />
a syncytium, but after infection a remarkable reaction occur in these cells. The cells<br />
line up in almost a single row just below the outer limiting border of the epidermis.<br />
Vacuoles appear in the cytoplasm of the epidermal cells, while <strong>org</strong>anelles such as<br />
mitochondria <strong>and</strong> Golgi apparatus are not anymore discernable.<br />
In a search for control agents of the citrus red mites (CRM) in Israel, field<br />
collected mite cadavers were examined for the presence of pathogens. This has<br />
resulted in the finding of three species of fungi that were found to be associated with<br />
mites. The fungi were described <strong>by</strong> Boekhout et al. (2003) as novel species<br />
belonging to the Ustilagomycetes, a class that is also called the smut fungi. It is a<br />
large taxon with over 1,400 species in 70 genera that are almost exclusively plant<br />
pathogens. The three fungi are anamorphic (they have no sexual state) <strong>and</strong> belong<br />
therefore to the Deuterymycetes. However, morphologically they are similar to<br />
yeast-like fungi which have been classified in the Ustilaginales. Based on molecular<br />
properties, they should be considered to belong to two different lineages within the<br />
Exobasidiomycetidae of the Ustilaginomycetes (Basidiomycota). These fungi,<br />
described as Meira geulakonigii, M. argovae <strong>and</strong> Acaromyces ingoldii, are hard to<br />
isolate from field-collected material: they are slow-growing fungi <strong>and</strong> for their<br />
identification physiological <strong>and</strong> molecular methods are needed. This probably<br />
explains the fact that they have only recently been discovered.<br />
The three fungi were further studied with respect to their potential as biological<br />
control agents of phytophagous mites. Laboratory investigations showed that all<br />
three fungi affected mites, although M. argovae showed no effect towards T. urticae.<br />
(Gerson et al., 2008). Meira geulakonigii caused considerable mortality of spider<br />
mites <strong>and</strong> citrus red mite. An interesting observation was that none of the fungi<br />
invaded the mites, although the fungi did grow on the mite’s cadavers. It is assumed<br />
that mortality among the mites was caused <strong>by</strong> the action of fungal toxins.<br />
Further tests showed that the fungus was endophytically present within the<br />
sealed grapefruit flowers <strong>and</strong> in the flavedo (the tough outer skin) of grapefruit.<br />
There was no evidence that the fungus caused any damage to the plants, which led<br />
the authors to the assumption that M. geulakonigii serves as a “body guard” of<br />
grapefruits. Also, M. geulakonigii had only minimal fungicidal effect on some<br />
predatory mites. This property, together with its tolerance to many insecticides <strong>and</strong><br />
acaricides, suggests that this fungus has possibilities for integrated control programs.<br />
4.3. Ascomycota<br />
The Ascomycota is a large taxon of fungi with approximately 2,000 genera <strong>and</strong> over<br />
30,000 species. Members of the Ascomycota bear the sexual spores within an ascus,<br />
originally a cell that at first contains a diploid nucleus resulting from karyogamy (the
286<br />
L.P.S. VAN DER GEEST<br />
fusion of nuclei or nuclear material that occurs during sexual reproduction). The<br />
nucleus undergoes subsequently meiosis, resulting in the formation of haploid<br />
ascospores inside the asci. These asci are often borne in or on top of a sporocarp.<br />
Very few Ascomycota have been isolated from mites. These isolations concern<br />
mainly Laboulbeniales infections in a number of mite species. Laboulbeniales is an<br />
order of fungi with more than 2,000 species. They are small, often minute fungi that<br />
have an obligate association with arthropods, mainly insects, <strong>and</strong> they lack<br />
mycelium. On their host, they appear as scattered or densely crowded bristles or<br />
bushy hairs which may form furry or velvety patches on certain part of the host’<br />
integument. These plume-like structures <strong>and</strong> triggers help in ascospore release when<br />
the arthropod comes into contact with a mature thallus.<br />
The site of attachment is usually limited to definite regions on the integument of<br />
each host. The entire thallus (body) is derived from enlargement <strong>and</strong> subsequent cell<br />
division of the two-celled ascospore. Below the surface of the arthropod cuticle<br />
absorption through a peg- or root-like haustorium provides a nutrition source for the<br />
fungus; however, the fungal parasites of this group do not appear to cause much<br />
damage to the host. A few species have been found on mites, including a Rickia sp.<br />
<strong>and</strong> an unknown species on Hirstionyssus (Demanyssidae) (Steinhaus & Marsh, 1962).<br />
5. DISEASES CAUSED BY EUKARYOTIC MICROPARASITES<br />
Traditionally, the animal kingdom has been divided into two subkingdoms: the<br />
Protozoa (unicellular eukaryotes) <strong>and</strong> the Metazoa (multicellular animals). In<br />
modern taxonomy, a kingdom Protista is considered of which the members are either<br />
unicellular, colonial or multicellualar. All these <strong>org</strong>anisms are eukaryotes,<br />
The Protista are divided into three major groups: the Protozoa, the Algae <strong>and</strong><br />
the Fungus-like protists. Protozoa are defined as single-celled eukaryotic <strong>org</strong>anisms,<br />
that feed heterotrophically (feeding both on both <strong>org</strong>anic <strong>and</strong> in<strong>org</strong>anic raw<br />
materials) <strong>and</strong> exhibit diverse motility mechanisms. Traditionally, four divisions are<br />
discerned, based on their mode of mobility:<br />
- Flagellata (Mastigophora) are protozoa that move <strong>by</strong> means of flagellar<br />
action. Some flagellates have their flagella attached in a structure called an<br />
undulating membrane. They often have symbiotic relationships with<br />
multicellular <strong>org</strong>anisms.<br />
- Rhizopoda (Amoebozoa) Rhizopoda are protozoa that move <strong>by</strong> employing<br />
pseudopodia, which are covered <strong>by</strong> membranes. These pseudopodia are<br />
cytoplasmic extensions that are not only used for locomotion but also to<br />
engulf food. Amoebae live in moist terrestrial <strong>and</strong> aquatic environment.<br />
- Apicomplexa (or Sporozoa). The Sporozoa are parasitic spore formers that<br />
do not move <strong>by</strong> their own power. Plasmodium vivax, the cause of malaria,<br />
is a sporozoan.<br />
- Ciliata (Ciliophora) Ciliata are protozoa that move <strong>by</strong> means of cilia action.<br />
Cilia are small <strong>and</strong> numerous; flagella are large <strong>and</strong> few. Because of the<br />
tremendous variety in ciliary arrangements <strong>and</strong> functions, ciliates are<br />
among the most diverse cells in the biological world.
MITE PATHOGENS IN IPM 287<br />
Table 4. Protozoan infections in mites.<br />
Species Mite host Mite family References<br />
Apicomplexa<br />
Acarogregarina<br />
corolla<br />
Scutovertex minutus Scutoverticidae Erhardová (1955)<br />
Asterophora<br />
caloglyphi<br />
Erhardovina<br />
bisphaera<br />
Caloglyphus moniezi Acaridae Geus (1969)<br />
Damaeus clavipes Damaeidae Purrini <strong>and</strong> Ormieres<br />
(1981)<br />
Damaeus onustus Damaeidae Purrini <strong>and</strong> Ormieres<br />
(1981)<br />
Eupelops hirtus Eupelopidae Purrini <strong>and</strong> Ormieres<br />
(1981)<br />
E. carabodesi Carabodes coriaceus Carabodidae Purrini <strong>and</strong> Ormieres<br />
(1981)<br />
E. euzeti Euzetes seminulum Euzetidae Lipa (1982)<br />
E. fuscozetesi Fuscozetes setosus Ceratozetidae Purrini, Bukva, <strong>and</strong><br />
Bäumler (1979)<br />
E. fuscozetesi Euzetes globulus Euzetidae Purrini <strong>and</strong> Ormieres<br />
(1981)<br />
E. oribatarum Mite see Lipa (1971)<br />
E. phtiracari Phthiracarus globosus Phthiracaroidea Purrini <strong>and</strong> Ormieres<br />
(1981)<br />
Phthiracarus piger Phthiracaroidea Purrini <strong>and</strong> Ormieres<br />
(1981)<br />
E. platynothri Platynothrus peltifer Nothroidea Purrini <strong>and</strong> Ormieres<br />
(1981)<br />
E. postneri Hermannia gibba Hermannioidea Purrini et al. (1979)<br />
E. scutovertexi Scutovertex minutus Scutoverticidae Erhardová (1955)<br />
Erhardovina sp. Limnochares aquatica Hydrachnellae Issi <strong>and</strong> Lipa (1968)<br />
Gregarina sp. Eupelops subuliger Eupelopidae Purrini et al. (1979)<br />
Eupelops torulosus Eupelopidae Purrini et al. (1979)<br />
Rhysotritia ardua Phthiracaroidea Purrini et al. (1979)<br />
Erhardovina sp. Damaeus geniculatus Damaeidae see Lipa (1971)
288<br />
L.P.S. VAN DER GEEST<br />
Table 4 Continued<br />
Erhardovina sp. Damaeus oblongus Damaeidae see Lipa (1971)<br />
Gurleya sokolovii Limnochares aquatica Hydrachnellae Issi <strong>and</strong> Lipa (1968)<br />
Unidentified<br />
gregarine<br />
Tyrophagus<br />
putrescentiae<br />
Acaridae Steiner (1993)<br />
Adelina acarinae Nothrus silvestris Nothroidea Purrini (1984)<br />
Microspora<br />
Intexta acarivora<br />
Tyrophagus<br />
putrescentiae<br />
Tyroglyphidae<br />
Larsson, Steiner, <strong>and</strong><br />
Bjørnson, (1997)<br />
Microsporidium<br />
phytoseiuli<br />
Phytoseiulus persimilis Phytoseiidae Bjørnson, Steiner,<br />
<strong>and</strong> Keddie (1996)<br />
Microsporidium sp. Amblyseius barkeri Phytoseiidae Beerling <strong>and</strong> Van der<br />
Geest (1991a, 1991b)<br />
Neoseiulus<br />
cucumeris<br />
Phytoseiidae<br />
Beerling <strong>and</strong> Van der<br />
Geest (1991a; 1991b)<br />
Napamichum<br />
aequifolium<br />
Limnochares aquatica Hydrachnellae Larsson (1990)<br />
Nosema acari Damaeus onustus Damaeidae Purrini <strong>and</strong> Weiser<br />
(1981)<br />
Damaeus clavipes Damaeidae Purrini <strong>and</strong> Weiser<br />
(1981)<br />
N. euzeti Euzetes seminulum Euzetidae Lipa (1982)<br />
N. führeri Phthiracarus globosus Phthiracaroidea Purrini & Weiser<br />
(1981)<br />
N. helminthorum Ceratoppia sp. Liacaroidea Moniez (1887)<br />
Ceratoppia bipilis Liacaroidea Dissanaike (1958)<br />
Xenillus tegeocranus Liacaroidea Dissanaike (1958)<br />
N. hermanniae Hermannia gibba Hermannioidea Purrini et al. (1979)<br />
N. ptyctimae Rhysotritia ardua Phthiracaroidea Purrini <strong>and</strong> Bäumler<br />
(1976)<br />
N. sperchoni Sperchon sp. Sperchontidae Lipa (1962)<br />
N. steganacari Steganacarus striculus Phthiracaroidea Purrini <strong>and</strong> Weiser<br />
(1981)
MITE PATHOGENS IN IPM<br />
289<br />
Table 4 Continued<br />
N. steinhausi Tyrophagus putrescentiae Tyroglyphidae Weiser (1956)<br />
Oligosporidium<br />
occidentalis<br />
Metaseiulus occidentalis Phytoseiidae Becnel, Jeyaprakash,<br />
Hoy, <strong>and</strong> Shapiro<br />
(2002)<br />
Pleistophora cephei Cepheus dentatus Cepheoidea Purrini <strong>and</strong> Weiser<br />
(1981)<br />
P. dindali Carabodes coriaceus Carabodidae Purrini <strong>and</strong> Weiser<br />
(1981)<br />
P. platynothri Platynothrus peltifer Nothroidea Purrini <strong>and</strong> Weiser<br />
(1981)<br />
P. oribatei Carabodes femoralis Carabodidae Purrini <strong>and</strong> Weiser<br />
(1981)<br />
Damaeus clavipes Damaeidae Purrini <strong>and</strong> Weiser<br />
(1981)<br />
Microtritia minima Euphthiracaroidea Purrini <strong>and</strong> Weiser<br />
(1981)<br />
Phthiracarus piger Phthiracaroidea Purrini <strong>and</strong> Weiser<br />
(1981)<br />
Phthiracarus sp. Phthiracaroidea Purrini <strong>and</strong> Weiser<br />
(1981)<br />
Physotritia duplicata Phthiracaroidea Purrini <strong>and</strong> Weiser<br />
(1981)<br />
Thelohania<br />
microtritiae<br />
Microtritia minima Euphthiracaroidea Purrini <strong>and</strong> Weiser<br />
(1981)<br />
The above classification is still being used, but we know now on the basis of<br />
ribosomal RNA gene sequencing that various groups in the Flagellata <strong>and</strong> Rhizopoda<br />
are not closely related. There may be greater genetic difference between two groups of<br />
Flagellata than between flowering plants <strong>and</strong> vertebrates. In modern classification, the<br />
following seven phyla are distinguished: Apicomplexa, Sarcomastigophora,<br />
Microspora, Ciliophora, Acetosphora, Myxospora <strong>and</strong> La<strong>by</strong>rinthomorpha. It is not<br />
within the scope of this chapter to go into details about this classification.<br />
Two phyla of the subkingdom Protozoa, the Apicomplexa <strong>and</strong> the Microspora,<br />
have members that are found in arthropods. Some of these are also pathogens of<br />
vertebrates, while others are commensals or weak pathogens; sometimes, they are<br />
highly virulent <strong>and</strong> pathogenic <strong>org</strong>anisms (cf. Tanada & Kaya, 1993).<br />
Protozoa associated with mites are mainly found in the Apicomplexa, with the<br />
classes Gregarina <strong>and</strong> Coccidia, <strong>and</strong> in the phylum Microspora. The class Gregarina<br />
is divided into the orders Eugregarinida <strong>and</strong> Neogregarinida. Several members of the<br />
former order have been detected in mites.
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The phylum Microspora also contains several pathogens of mites. Table 4 lists<br />
protozoan species that have hitherto been isolated from mites. There is little<br />
information available on the population dynamical effects of these <strong>org</strong>anisms on<br />
natural mite populations.<br />
5.1. Apicomplexa Infections in Mites<br />
Apicomplexans have very complex life cycles, with much variation among the<br />
different apicomplexan groups. Both asexual <strong>and</strong> sexual reproduction is involved,<br />
although some Apicomplexa skip one or the other stage. The life cycle starts when<br />
an infective stage, the sporozoite, enters a host cell, <strong>and</strong> then divides repeatedly to<br />
form numerous merozoites. Some of the merozoites transform into sexually<br />
reproductive cells, or gamonts. These gamonts join together in pairs <strong>and</strong> form a<br />
gamontocyst. Within the gamontocyst, the gamonts divide to form numerous<br />
gametes. Pairs of gametes then fuse to form zygotes, which give rise <strong>by</strong> meiosis to<br />
new sporozoites, <strong>and</strong> the cycle starts all over again.<br />
Apicomplexa are transmitted to new hosts in various ways; some, like the<br />
malaria parasite, are transmitted <strong>by</strong> infected mosquitoes, while others may be<br />
transmitted in the feces of an infected host, or when a predator eats infected prey.<br />
Gregarinia, or gregarines have mature gamonts (trophozoites) that are large <strong>and</strong><br />
extracellular. The gamonts are found in the digestive tract <strong>and</strong> body cavities of<br />
invertebrates <strong>and</strong> they possess <strong>org</strong>anelles (see Tanada & Kaya, 1993). They have<br />
usually similar gametes (isogametes) <strong>and</strong> undergo syzygy: mature gamonts detach<br />
themselves from the midgut <strong>and</strong> line themselves end to end in pairs or in large<br />
numbers to form a prenuptial association. The zygotes form oocysts within<br />
gametocysts. Eugregarines have a life cycle that consists only of gametogony <strong>and</strong><br />
sporogony, but the neogregarines, considered more primitive, have an additional<br />
schizogony (a multiple fission process). This schizogony (or merogony) occurs<br />
intra- or extracellularly <strong>and</strong> causes the presence of larger numbers of the pathogen<br />
than in case of the eugregarines. These higher numbers result in a more virulent<br />
infection.<br />
As early as 1885, the eugregarine Gregarina oribataram was reported in an<br />
unidentified mite (see Lipa, 1971). Unidentified gregarine infections were observed<br />
in the oribatids Damaeus oblongus <strong>and</strong> D. geniculatus (Damaeidae) <strong>by</strong> Michael in<br />
1884 <strong>and</strong> Wellmer in 1911 (see Lipa, 1971). Gregarina scutovertexi was described<br />
<strong>by</strong> Erhardová in 1955 from Scutovertex minutus, an oribatid mite that serves as<br />
vector of the tape worm Monieza expansa. Several other eugregarine species were<br />
described <strong>by</strong> Purrini et al. (1979) <strong>and</strong> Purrini <strong>and</strong> Ormiers (1981). For more details<br />
is referred to Table 4.<br />
An interesting eugregarine infection was also noted in the intestinal wall of the<br />
water mite Limnochares aquatica (Hydrachnellidae) (see Issi & Lipa, 1968), while<br />
Gregarina euzeti was detected in the oribatid Euzetes seminulum (Lipa, 1982).<br />
Despite all these reports on gregarines, no data are available on the impact of these<br />
infections on the host. It is generally believed that gregarines are of low virulence.
MITE PATHOGENS IN IPM<br />
291<br />
Coccidia differ from the gregarines in their gamogony: female gamonts of<br />
gregarines give rise to a number of gamonts whereas those of Coccidea only to<br />
single gamonts. One coccidian species has been described from an oribatid (Purrini,<br />
1984).<br />
5.2. Microspora Infections in Mites<br />
Microspora (or Microsporidia) are obligate intracellular parasites with a broad host<br />
range including all animal groups. They rank among the smallest eukaryotes (1–40 μm)<br />
with the shortest eukaryotic genome <strong>and</strong> are generally considered to be a separate<br />
phylum within the subkingdom Protozoa. However, recent molecular studies<br />
indicate that they may be considered to be extremely reduced fungi. Replication<br />
takes place within the host's cells, which are infected <strong>by</strong> means of unicellular spores.<br />
Microsporidia are unusual in lacking mitochondria <strong>and</strong> in having mitosomes. 4<br />
They also lack motile structures such as flagella. The spores are protected <strong>by</strong> a<br />
layered wall made of proteins <strong>and</strong> chitin. Their interior is dominated <strong>by</strong> a unique<br />
coiled structure called the polar filament. Spores, the infective stage, are ingested <strong>by</strong><br />
the host <strong>and</strong>, in the midgut, their polar filament is instantaneously emitted as turning<br />
a garden hose inside out. The polar tube penetrates the host cell <strong>and</strong> the contents of<br />
the spore are pumped through it without destruction of the host cell. Within the host<br />
cell, an increase in numbers followed <strong>by</strong> the development into new spores takes<br />
place. In this way, the infection spreads throughout the host. Many different tissues<br />
may be affected. The spores may be released into the environment during the life of<br />
the host or after its death. The spores are the only stages that can survive outside the<br />
host. Many microsporidia have very complex life cycles with several spore types<br />
<strong>and</strong> host involved. Microsporidiosis is often transmitted vertically (from mother to<br />
offspring), usually without spores as intermediary. Vertical transmission may be<br />
transovarial, <strong>by</strong> passage though the ovary, or transovum, a form of transovarial<br />
transmission in which the pathogen enters the egg while it is still in the ovary.<br />
Taxonomy was in the past mainly based on spore size <strong>and</strong> shape. These<br />
characters are, however, unsatisfactory <strong>and</strong> for that reason, ultrastructural<br />
characteristics have been used. This has caused a considerable revision in this group<br />
of pathogenic <strong>org</strong>anisms (Sprague, Becnel, & Hazard, 1992). Recently, several<br />
research groups have started to integrate molecular techniques for phylogenetic<br />
studies of Microsporidia. This will undoubtedly result in a new revision of these<br />
taxa.<br />
The first microsporidium described in mites was Nosema steinhausi (Weiser,<br />
1956) from the stored product mite Tyrophagus putrescentiae (Tyroglyphidae). The<br />
disease affects both adults <strong>and</strong> nymphs. Experiments in a colony of the mite showed<br />
that the disease progressed from about 10% infection at the start of the experiment to<br />
4 A mitosome is an <strong>org</strong>anelle found in some unicellular eukaryotic <strong>org</strong>anisms. The<br />
mitosome has only recently been found <strong>and</strong> named, but its function has not yet been<br />
well characterized. It is sometimes termed a crypton.
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75% after 2 months. The colony was completely eradicated after a further 2 weeks.<br />
Several other authors have described microporidia from various species of mites.<br />
For more details refer to Table 4.<br />
In the late 1980s poor performance was noted of phytoseiids used as biological<br />
control agent for thrips <strong>and</strong> spider mites in greenhouse crops <strong>and</strong> this observation<br />
has led to studies on the possible involvement of pathogens in predator colonies.<br />
Beerling <strong>and</strong> Van der Geest (1991a, 1991b) studied a microsporidosis in mass<br />
cultures of the predators Amblyseius barkeri <strong>and</strong> Neoseiulus cucumeris<br />
(Phytoseiidae) that are being used for the control of the thrips pests Frankliniella<br />
occidentalis <strong>and</strong> Thrips tabaci (Thripidae) on vegetable <strong>and</strong> ornamental crops in<br />
greenhouses. Diseased predators show a low reproduction <strong>and</strong> predation capacity of<br />
the mites unsatisfactory. Predatory mites were sluggish in their movement <strong>and</strong> had a<br />
swollen <strong>and</strong> whitish appearance (Beerling & Van der Geest, 1991a).<br />
The presence of numerous spores could be detected in squash preparations of<br />
the mites <strong>and</strong> it was assumed, that the pathogen involved belonged to the<br />
Pleistophoridae (Microspora). Also infected stored product mites were observed.<br />
Further work showed that three different spore types are found in the predator<br />
cultures. It is difficult to say that three species of Microsporidia are involved, since<br />
some species have several spore types during their life cycle. Recently, a new<br />
species of a microsporidium parasite, Intexta acarivora, was observed in the gut<br />
epithelium of the forage mite T. putrescentiae (Larsson et al., 1997), obtained from a<br />
commercial culture in The Netherl<strong>and</strong>s. Mites of this culture are used as prey for a<br />
commercial rearing of N. cucumeris.<br />
Beerling <strong>and</strong> Van der Geest (1991a, 1991b) also studied infected mite strains<br />
from a commercial rearing in The Netherl<strong>and</strong>s, but it is not known whether this has<br />
the same origin as the samples studied <strong>by</strong> Larsson et al. (1997). The spore size<br />
values of this microsporidium do not correspond with any of the values of the spores<br />
in Beerling, Rouppe van der Voort, <strong>and</strong> Kwakman (1993).<br />
Bjørnson et al. (1996) studied colonies of P. persimilis that were obtained from<br />
suppliers of biological control agents. On the basis of spore morphology, three<br />
distinct microsporidia could be observed in strains of P. persimilis, obtained from<br />
three different suppliers. The ultrastructure of the pathogen <strong>and</strong> the course of the<br />
disease of a colony obtained from Europe were studied in more detail. Schizonts<br />
were observed inside the nuclei of the digestive cells of the ventriculus <strong>and</strong> within<br />
the protoplasm of cells that line the caecal wall <strong>and</strong> the muscle tissue underlying it.<br />
The properties of the pathogen made it difficult to assign it to an existing genus. For<br />
that reason, it was placed in the collective group Microsporidium. Vertical<br />
transmission for this microsporidium was proven, as mature spores were observed in<br />
developing eggs inside gravid females (Fig. 11). The performance of an infected<br />
colony was greatly affected (Bjørnson & Keddie, 1999): mean fecundity <strong>and</strong> prey<br />
consumption of infected mites were significantly reduced. Short-term survivability<br />
was variable <strong>and</strong> was not a good measure of predator quality. However, uninfected<br />
females lived longer than infected females.
MITE PATHOGENS IN IPM<br />
293<br />
Figure 11. Cross section of a microsporidian spore <strong>and</strong> a crystal of Phytoseiulus<br />
persimilis. The polar filament of the spore is not visible. Photograph <strong>by</strong> Dr. Susan<br />
Bjørnson.<br />
Poor performance of the predators, due to the presence of pathogens in the mass<br />
cultures is a threat to integrated pest management in especially glasshouse crops<br />
(e.g. Steiner, 1993). It is clear that more attention should be paid to a good<br />
monitoring system. The presence of pathogens should be established early in the<br />
manufacturing process, which requires a fast <strong>and</strong> reliable detection method. In the<br />
past, visual inspection with the aid of a binocular or compound microscope was the<br />
only way to establish the presence of these pathogens. A polarizing filter is needed<br />
to avoid confusion with the birefringent crystals that are commonly present inside<br />
adult phytoseiids (see Section 6.1).<br />
The availability of a method to detect the disease at an early stage is of great<br />
importance for the commercial production of natural enemies. Beerling et al. (1993)<br />
developed an ELISA to detect the presence of microsporidiosis in predator massrearings.<br />
Monoclonal antibodies were produced against one spore type (oblong), that<br />
was present in both prey <strong>and</strong> predator species. A next step would be the use of more<br />
sensitive molecular techniques which makes the detection of microsporidiosis<br />
possible regardless of spore type, <strong>and</strong> even before spores are formed (Malone &<br />
McIvor, 1996).<br />
Recently, a new species of microsporidia was described <strong>by</strong> Becnel, Jeyaprakash,<br />
Hoy, <strong>and</strong> Shapiro (2002) from the predatory mite Metaseiulus occidentalis. Mites<br />
infected with Oligosporidium occidentalis do not show any external or gross signs<br />
of infection, but electronmicroscopical analysis reveales that the pathogen develops<br />
in eggs, larvae, nymphs <strong>and</strong> adults of the predator. Mature cells of O. occidentalis can<br />
be found in cecal cells, lyrate <strong>org</strong>an cells, ganglia, epithelial cells, muscle, inside the<br />
ovary <strong>and</strong> in developing <strong>and</strong> mature eggs. Female predators have in general a shorter
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life span, a low oviposition rate <strong>and</strong> fewer female progeny. No effect could be<br />
shown on longevity of males or on male progeny survival to larval <strong>and</strong> adult stages.<br />
The infection may affect the performance of the predator. Heat treatments of<br />
infected colonies had some success: eggs placed for 7 days in a chamber at 33°C <strong>and</strong><br />
subsequently at 27°C showed a reduced infection rate, but the disease was still not<br />
completely eliminated. Mites emerging from these eggs still showed spores inside<br />
their body, but it was assumed that most of these spore were dead as the majority of<br />
the mites survived. After a number of weeks, infection rates were again high,<br />
indicating that the heat treatment was only partially effective. However, when eggs<br />
were placed at 33°C. <strong>and</strong> when their progeny was also kept at this temperature,<br />
disease-free mites were obtained. It was also shown that the disease may be<br />
horizontally transmitted, probably <strong>by</strong> cannibalism.<br />
At this moment, no other cure exists for microsporidiosis in predatory mite<br />
mass rearings. Anti-microsporidial compounds, such as albendazole, fumagillin,<br />
metronidazole <strong>and</strong> nifedipine were not successful in eliminating microsporidiosis in<br />
mass cultures of P. persimilis (Bjørnson, 1998). Therefore, efforts should be made to<br />
keep the starting cultures of predatory mites disease-free. Heat treatment of infected<br />
eggs, or rearing infected individuals at elevated temperatures, has been shown to<br />
reduce disease prevalence in some cases; however, the most effective <strong>and</strong> practical<br />
means for rearing microsporidian free predatory mites is to start a new rearing with<br />
progeny from uninfected females.<br />
6. OTHER DISEASES<br />
6.1. Symptoms Ascribed to Poor Condition<br />
In this chapter, we discuss a condition in mites that cannot be ascribed to the action<br />
of a pathogen. In a number of instances, rectal plugs, usually in combination with<br />
abdominal discoloration have been observed in phytoseiids (Tanigoshi, Fagerlund,<br />
& Nishio-Wong, 1981; Bjørnson et al., 1997). This discoloration is usually<br />
manifested as two white stripes along the dorsal sides of the body within the<br />
Malpighian tubules. The condition is frequently found in laboratory colonies of<br />
predatory mites <strong>and</strong> it may be a sign of poor condition of the predator. Tanigoshi<br />
(1982), for example, considered the condition a sign of senescence. Affected mites<br />
are often lethargic <strong>and</strong> have frequently numerous densely packed, birefringent<br />
dumbbell-shaped bodies, mainly in the Malpighian tubules, rectum <strong>and</strong> anal atrium.<br />
In Cheyletus eruditus, abdominal discoloration is also associated with the<br />
occurrence of birefringent crystals in the excretory <strong>org</strong>ans, especially when reared<br />
under crowded conditions. These crystals are considered to be the normal excretory<br />
products (Hughes, 1950) <strong>and</strong> probably consist of guanine <strong>and</strong> uric acid (McEnroe,<br />
1961). These compounds are insoluble <strong>and</strong> are probably stored in the malpighian<br />
tubes prior to excretion. The crystals observed in P. persimilis, however, contain<br />
high levels of potassium, low levels of phosphorous <strong>and</strong> sulphur <strong>and</strong> traces of<br />
chlorine, very unlike the common waste products mentioned above (Bjørnson,<br />
1998). Large numbers of crystals in mites are especially found in laboratory mites,
MITE PATHOGENS IN IPM<br />
295<br />
reared under crowded condition (Fig. 12), <strong>and</strong> it is assumed that they are an<br />
indication of a poor condition of the mites.<br />
Figure 12. Crystals in tissue of Phytoseiulus persimilis. Such crystals are often an<br />
indication of a poor condition of the mite. Photograph of Dr. Susan Bjørnson.<br />
6.2. Identification of Pathogens<br />
Recognition of an <strong>org</strong>anism causing disease in noxious mites will aid in the process<br />
of implementing control strategies against such mites, while it will also be of great<br />
importance to know disease causing <strong>org</strong>anisms in mites that are mass reared for<br />
biological control purposes. However, identification of pathogens is not in all<br />
instances easy: for example, virus recognition in diseased mites may require very<br />
comprehensive research before one may decide that a virus is the disease causing<br />
agent. In contrast to insects, very few viruses have been isolated from mites <strong>and</strong> the<br />
viruses known to cause disease in mites are not as readily identifiable as some of the<br />
insect viruses. A large number of insect viruses belong to the baculoviruses, rodshaped<br />
viruses that may form large inclusion bodies (polyhedra) in the cell nuclei<br />
(nuclear polyhedrosis viruses), or smaller so-called granula (granulosis viruses).<br />
Other viruses, the cytoplasmic polyhedrosis viruses are icosahedra <strong>and</strong> are also<br />
included in large inclusion bodies of irregular form. Identification of such viruses<br />
can partially be done <strong>by</strong> light-microscopic means, in combination with more<br />
sophisticated molecular techniques. Such viruses are not known from Acari.<br />
Hitherto, only few viruses have been identified as pathogen of mites.<br />
Bacteria causing disease are often obligate intracellular <strong>org</strong>anisms. Classical<br />
identification based on characters such as nutrient requirement <strong>and</strong> structure of<br />
colonies on artificial media is not possible as these bacteria cannot be grown outside<br />
it host’s cell. However, the availability of molecular techniques has made
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L.P.S. VAN DER GEEST<br />
identification of such intracellular bacteria possible <strong>by</strong>, among others, analysis of<br />
16S rDNA gene sequences. The best-known species of such intracellular bacteria<br />
belong to the genus Wolbachia, probably the most widely-spread parasitic bacterium<br />
known. Abnormal sex ratios, incompatibilities between strains of mites <strong>and</strong> absence<br />
of male offspring may point to the presence of Wolbachia sp. or other symbionts.<br />
Feeding infected mites with antibiotics may remove these parasitic bacteria <strong>and</strong> will<br />
result in “normal” offspring. Molecular analysis of 16S rDNA will finally prove the<br />
presence of Wolbachia or other intracellular bacteria.<br />
The largest number of pathogens of mites is found in the fungi. Pathogens of<br />
mites are mainly found in the Zygomycota <strong>and</strong> Deuteromycota (or Fungi<br />
Imperfecti). For a proper identification, it is usually necessary to study sporulating<br />
fungi. This can be accomplished <strong>by</strong> incubating the infected mites under conditions<br />
of a high relative humidity.<br />
Zygomycota are characterized <strong>by</strong> the absence of cross walls (septa) in their<br />
hyphae <strong>and</strong> the presence of tick-walled, sexual spores (zygospores). However, the<br />
primary taxonomic emphasis is on asexual reproductive structures. The asexual<br />
spores (conidia) are released from the conidiophores <strong>by</strong> force <strong>and</strong> form often a halo<br />
around the host’s cadaver. Species infecting mites form secondary conidia upon<br />
germination of these conidia. The secondary conidium is much smaller in size <strong>and</strong> is<br />
called capilliconidium. Identification to the species is often difficult <strong>and</strong> requires the<br />
aid of specialists. Of some species, only zygospores (or resting spores) are known.<br />
Taxonomy of these species is mainly based on the properties of these spores. These<br />
species have been lumped together in the genus Tarichium.<br />
Several Deuteromycetes have been isolated from Acari, belonging to the<br />
following genera: Aspergillus, Beauveria, Cephalosporium, Hirsutella,<br />
Paecilomyces, Sporothrix, Tolypocladium <strong>and</strong> Lecanicillium (Verticillium). A key to<br />
the genera of Deuteromycetes infecting insects <strong>and</strong> mites can be found in Samson<br />
(1981). Identification requires examination of conidium ontogeny which is the<br />
primary character for typifying the different genera. There are two modes of blastic<br />
conidiogenesis: phialidic <strong>and</strong> sympodal. A succession of conidia is produced <strong>by</strong> a<br />
phialidic conidiogenous cell. The shape of the phialide is dependent on the genus:<br />
flask-like in Paecilomyces <strong>and</strong> Hirsutella, awl-like in Lecanicillium <strong>and</strong> cylindrical<br />
in Metarhizium. The conidia are produced in chains (Paecilomyces, Metarhizium), or<br />
they are contained in slimy heads or droplets (Lecanicillium, Fusarium). Phialides of<br />
Hirsutella form conidia that are held together in a slimy sheath. This gives the<br />
impression that only one conidium is being produced. Sympodial development is<br />
observed in species of the genera Beauveria <strong>and</strong> Sporothrix. Conidia are formed<br />
singly on a laterally proliferating conidiogenous cell that often shows a geniculate or<br />
zigzag type of elongation. For more details is referred to Samson (1981).<br />
7. PROSPECTS OF ACAROPATHOGENS FOR INTEGRATED PEST<br />
MANAGEMENT<br />
Comprehensive research has been conducted to study the possibilities to use<br />
pathogens for the control of insects <strong>and</strong> other invertebrate pests. There are several<br />
cases known how pathogens may decimate populations of phytophagous mites under
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297<br />
natural conditions. An early example is a virus disease of the citrus red mite in citrus<br />
groves throughout California <strong>and</strong> Arizona (Reed, 1981). However, successful<br />
application of the virus failed for a variety of reasons. Mass production of the virus<br />
is difficult as the virus can only be grown in living mites. This fact makes mass<br />
production very laborious <strong>and</strong> expensive. Furthermore, the virus becomes rapidly<br />
inactivated <strong>by</strong> sunlight when applied in aqueous formulations, while high<br />
temperatures, common in citrus orchards in California <strong>and</strong> Arizona, also have a<br />
negative effect on the virulence of the virus. Inactivation of the virus <strong>by</strong> sunlight<br />
may be overcome <strong>by</strong> the addition of ultraviolet protecting substances. The main<br />
reason that this virus, although very host specific, has never been successful are the<br />
difficulties encountered during mass production. Biological acaricides with viruses<br />
as active ingredient are not foreseen for the near future, as few viruses of<br />
phytophagous mites are known. The situation with respect to the varroa mite Varroa<br />
jacobsoni may be completely different. Several viruses have been isolated from this<br />
parasitic mite <strong>and</strong> more research may lead to the discovery of viruses that could be<br />
used for the control of the varroa mite. A point to worry about is that the varroa mite<br />
may act as vector of honey bee viruses. Host specificity experiments are for that<br />
reason of great importance.<br />
Many fungal pathogens show a high pathogenicity towards phytophagous mites.<br />
There are several examples showing how fungi are able to cause large epidemics in<br />
natural populations of tetranychids <strong>and</strong> eriophyids. One of the main obstacles for a<br />
successful application of fungal pathogens for the control of invertebrate pests in<br />
agricultural crops is the ambient condition within the vegetation. Almost all fungi<br />
require a relative humidity near the saturation point for both spore germination <strong>and</strong><br />
spore formation. Entomophthorales epidemics have frequently been observed in<br />
insect <strong>and</strong> mite populations: Neozygites floridana is a fungal pathogen that may<br />
cause large reductions in population sizes of several species of spider mite. Such<br />
epidemics usually occur later in the season, when population sizes of spider mites<br />
are large <strong>and</strong> when relative humidity is near the saturation point. Damage to the crop<br />
has then already been inflicted.<br />
Experiments have been conducted to advance epidemics <strong>by</strong> inundative releases<br />
of the pathogen. The high virulence against certain target pests <strong>and</strong> their high<br />
specificity make these fungi attractive for inundative releases. However,<br />
entomophthoralean species are very fastidious: culturing <strong>and</strong> sporulation in artificial<br />
media is hardly possible which makes mass production of these fungi very<br />
expensive <strong>and</strong> laborious, as they should be grown in living mites. In addition, the<br />
infective stages of these fungi are rather short-lived <strong>and</strong> this characteristic makes<br />
their application difficult. It has been suggested that the use of these fungi in<br />
greenhouses may show good prospects (Maniania, Bugeme, Wekesa, Delalibera, &<br />
Knapp, 2008).<br />
In many greenhouses, high value horticultural crops are grown where<br />
environmental coniditions that normally favor the efficacy of these fungi can easier<br />
be manipulated than in outdoor crops. In addition, horizontal transmission of the<br />
fungus may be more efficient when spider mites densities are sufficiently high,<br />
making repeated inundative releases unnecessary. However, low spider mite<br />
densities would be an disadvantage for successful control of the pest concerned.
298<br />
L.P.S. VAN DER GEEST<br />
From the other h<strong>and</strong>, classical biological control with these fungi seems to be<br />
attractive in certain circumstances. Efforts have been made to use Neozygites<br />
tanajoae as a control agent for the cassava green mite in Africa <strong>by</strong> releasing the<br />
fungus in cassava fields in Benin as a classical biological control agent. The fungus<br />
has later been isolated from the release areas where it caused a higher mortality<br />
among cassava mites than the local strains of N. tanajoae did. However, more<br />
knowledge is required. We know too little how the fungus overcomes unfavorable<br />
periods, about the role of resting spores <strong>and</strong> under which conditions may resting<br />
spores sporulates. Interesting observations were made <strong>by</strong> Elliot et al. (2008) in a<br />
cassava field in the state on Bahia, Brazil. Epidemics of the fungus were virtually<br />
absent when cassava green mite populations reached high densities, as not sufficient<br />
fungus inoculum was present. Later in the season, sufficient fungus inoculum was<br />
observed, but at that time no mites were present due to defoliation of the cassava<br />
plants. It is very hard to manipulate such a system, as mass production, followed <strong>by</strong><br />
inundative releases is impossible at a large scale.<br />
The fungus does not seem to be the solution for the cassava green mite problem<br />
in Africa, although it is promising that the fungus seems to become established in<br />
the release areas. The fungus may be an important factor in the control of the<br />
cassava mite, when applied in combination with predatory mites. A point of concern<br />
is also the use of chemical pesticides: it is known that, in particular fungicides may<br />
have a detrimental effect on the fungal pathogen. Careful selection of chemicals<br />
used in a crop system is of utmost importance.<br />
Figure 13. Brevipalpus phoenicis infected <strong>by</strong> Lecanicillium (Verticillium) lecanii.<br />
Photograph courtesy of Dr. Marcel Tanzini.<br />
Several Deuteromycota are known with a high virulence towards mites <strong>and</strong><br />
other invertebrates. This group of fungi can in general be grown in artificial media<br />
<strong>and</strong> mass production is therefore no problem. The first attempt to control an
MITE PATHOGENS IN IPM<br />
299<br />
invertebrate pest with a fungus of this group was already conducted in Russia in<br />
1888, when Krassilstschik sprayed a suspension of spores of Metarhizium anisopliae<br />
in the field for the control of the sugar beet curculio Cleonis punctiventris (cf.<br />
Steinhaus, 1949). Since then, many attempts have been made to formulate<br />
mycopesticides, mainly for the control of insect pests (De Faria & Wraight, 2007).<br />
Until now, 171 products have been developed worldwide with entomo- <strong>and</strong><br />
acaropathogens as active ingredients. Of these, 129 products are still available. The<br />
number of products that have been developed for use against mites is small: only 17<br />
products are recommended for use against Acari. The main part of these pesticides<br />
contains B. bassiana as active ingredient, but four preparations are based on<br />
Lecanicillium sp. (formerly Verticillium lecanii) (Fig. 13). Many of these species<br />
have a broad host spectrum, like Beauveria bassiana <strong>and</strong> Metarhizium anisopliae.<br />
The genus Hirsutella contains several members with a high specificity towards<br />
mites. The best studied species is H. thompsonii, originally described from the citrus<br />
rust mite Phyllocoptruta oleivora. Acaricidal preparations with H. thompsonii as<br />
active ingredient were developed in the 1980s for the control of the citrus rust mite,<br />
but the production was discontinued because of instability of the product. It is<br />
hopeful to notice that the interest in the production of H. thompsonii based<br />
acaricides has recently been renewed in India, <strong>and</strong> in some Latin American<br />
countries, but now for the control of rust mites in coconut. This renewed interest has<br />
led in India to the production of a successful bio-acaricide.<br />
In Colombia, biopesticides have been developed that contain a mixture of<br />
invertebrate pathogens, e.g. Microbiol Completo contains B. bassiana, M.<br />
anisopliae, Nomuraea rileyi, Isaria fumosorosea <strong>and</strong> B. thuringiensis. It is<br />
recommended for the control of a variety of insect species <strong>and</strong> Acari. It is<br />
remarkable that in particular in Latin American countries, many bioinsecticides are<br />
being developed with fungal pathogens as active ingredients. The climatic<br />
conditions may be more suitable for the applications of such pesticides than, e.g. in<br />
Europe. As mentioned earlier, a major drawback in the use of fungi is their<br />
dependence on a high relative humidity during spores germination. Oily<br />
formulations seem to be a solution to this problem. Oily substances protect the<br />
spores against desiccation <strong>and</strong> allow sporulation at a somewhat lower relative<br />
humidity.<br />
Hirsutella thompsonii var. synnematosa has been introduced from Zimbabwe<br />
<strong>and</strong> H. thompsonii var. vinacea from North Carolina as classical biological control<br />
agents for the control of Eriophyes sheldoni <strong>and</strong> Phyllocoptruta oleivora in<br />
Argentina. Infection levels after release were high, but no information is available<br />
about their persistence. The project has been discontinued (cf. Maniania et al., 2008).<br />
A point of major concern in integrated control programs is the quality of<br />
biological control agents. Predatory mites have been used for several decades for the<br />
control of spider mites in horticultural <strong>and</strong> agricultural crops. Low performance of<br />
predators has revealed the presence of pathogens. For reviews is referred to Schütte<br />
<strong>and</strong> Dicke (2008), Bjørnson (2008) <strong>and</strong> Hoy <strong>and</strong> Jeyaprakash (2008). Microspora<br />
species have been causing problems in mass cultures of several species of<br />
Phytoseiidae, in particular Amblyseius barkeri <strong>and</strong> A. cucumeris, but they are also<br />
known to occur in Phytoseiulus persimilis <strong>and</strong> Metaseiulus occidentalis. Sanitary
300<br />
L.P.S. VAN DER GEEST<br />
measures <strong>and</strong> careful selection of uninfected lines of predatory mites are still the<br />
only solution to these problems. Acaricomes phytoseiuli is a bacterium that affects<br />
the behavior <strong>and</strong> predacious capacity of P. persimilis. This bacterium has not yet<br />
been encountered in mass rearings for the predator, but it will be clear that screening<br />
for such pathogens is necessary. Another group of bacteria that can cause<br />
considerable damage in mass cultures of beneficial mites <strong>and</strong> insects are Wolbachia<br />
sp., Cardinium sp., Spiroplasma sp. <strong>and</strong> other bacteria that affect sex ratios <strong>and</strong> that<br />
may cause incompatibilities between strains of the same species. This type of<br />
bacteria is widespread in mites <strong>and</strong> other vertebrates<br />
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Schütte, C., & Dicke, M. (2008). Verified <strong>and</strong> potential pathogens of predatory mites (Acari:<br />
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Selhime, A. G., & Muma, M. H. (1966). Biology of Entomophthora floridana attacking Eutetranychus<br />
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Shaw, J. G., Chambers, D. L., & Tashiro, H. (1968). Introducing <strong>and</strong> establishing the noninclusion virus<br />
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Shaw, J. G., Moffitt, C., & Sciven, G. T. (1967). Biotic potential of phytoseiid mites fed on virus-infected<br />
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Shen, M., Yang X., Cox-Foster, D., & Cui, L. (2005). The role of varroa mites in infections of Kashmir<br />
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Shi, W. B., Feng, M. G., & Liu, S. S. (2008). Sprays of emulsifiable Beauveria bassiana forkulation are<br />
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Sreerama Kumar, P. L., & Singh S. P. (2008). Enabling mycelial application of Hirsutella thompsonii for<br />
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Sreerama Kumar, P. (2006). Hirsutella thompsonii as a mycoacaricide for Aceria guerreronis on coconut<br />
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Acarology, August 2006. Amsterdam, The Netherl<strong>and</strong>s, p. 198.<br />
Sreerama Kumar, P., & Singh, S. P. (2001). Coconut mite in India: Biopesticicide breakthrough.<br />
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12<br />
IPM STRATEGIES THROUGH SPECIALIST AND<br />
GENERALIST PHYTOSEIIDS (ACARI,<br />
MESOSTIGMATA)<br />
SAURO SIMONI AND MARISA CASTAGNOLI<br />
Agricultural Research Council,<br />
Research Centre for Agrobiology <strong>and</strong> Pedology<br />
via di Lanciola 12/A, Cascine del Riccio,<br />
50125 Firenze, <strong>Italy</strong><br />
Abstract. The exploitation of natural enemies, especially the predaceous mites phytoseiids, has become a<br />
fundamental factor for IPM in integrated crop production in Europe <strong>and</strong> worldwide. In controlling<br />
harmful insect <strong>and</strong> mite species, various species/strains from this group of predators are commonly used<br />
<strong>and</strong> marketed. Intrinsic biological traits of phytoseiids allow their ranking in different life style types.<br />
These factors, together with their quick adaptability to face new emergencies (i.e. phytophagous <strong>and</strong><br />
exotic pests outbreaks <strong>and</strong> new environment or climatic conditions) confirm their role as a significant <strong>and</strong><br />
sustainable tool in biological control. In this chapter the foundations for a more intensive adoption of<br />
phytoseiids are underlined, including the enhancement <strong>and</strong> introduction of new strategies aiming at a long<br />
term <strong>and</strong> efficient pest control.<br />
1. INTRODUCTION<br />
The need to increase food availability hardly couples with better chances to limit<br />
plant pests in modern agriculture, <strong>and</strong> several actions aim worldwide at increasing<br />
crop production <strong>and</strong> facilitating food <strong>and</strong> commodities trade. These efforts include<br />
lengthening of the plant/crops seasonal life or strategies increasing the consistent<br />
uniformity of varieties <strong>and</strong> cultivars used which represent, in fact, useful factors for<br />
business at small time scale. However, these actions are not always suitable to<br />
prevent a multitude of pest infestations on a regional scale. Since pests are also<br />
persistently poised for plant invasion, preventive <strong>and</strong> early remedial pest<br />
management strategies <strong>and</strong> treatments are needed at regular time intervals, in almost<br />
any cropping system (Sparks, 1999; Jarvis, Mar., & Sears, 2006; Gerson &<br />
Weintraub, 2007).<br />
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A. <strong>Ciancio</strong>, K.G. Mukerji (eds.), Integrated Management of Arthropod Pests<br />
<strong>and</strong> Insect Borne Diseases, Integrated Management of Plant Pests <strong>and</strong> Diseases 5,<br />
DOI 10.1007/978-90-481-8606-8_12, © Springer Science+Business Media B.V. 2010
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Given the worldwide trend towards crops with high genetic uniformity, much of<br />
the biodiversity found in the context of agroecosystems is sustained <strong>and</strong> maintained<br />
<strong>by</strong> means of the marginal environments surrounding productive areas. Any loss of<br />
such diversity due to crop management choices reduces farmers capacities to cope<br />
with plant stress factors. These include biotic factors like extreme temperatures,<br />
drought <strong>and</strong> salinity (Wang, Vinocur, & Altman, 2003). Consequently, due to the<br />
synergies occurring among biotic <strong>and</strong> abiotic stress factors, the problems that much<br />
of the world population practicing subsistence agriculture has to face are also<br />
emphasized. Furthermore, <strong>and</strong> typically in plants that regularly shut down, periodic<br />
inspections <strong>by</strong> specialists involved in integrated pest management (IPM) are needed<br />
for monitoring (with related costs). On the other h<strong>and</strong>, in more intensive agricultural<br />
systems, crop production in field or under protected conditions, whether in climatecontrolled<br />
greenhouses <strong>and</strong> glasshouses or tunnels with little or no climate control, is<br />
increasing worldwide, due to market dem<strong>and</strong>, demographic pressure <strong>and</strong>/or<br />
unavailability of suitable environments. Although these last cropping systems are<br />
closed <strong>and</strong> relatively protected, they still remain vulnerable to known or invasive pests.<br />
The general <strong>and</strong> pressing consumers dem<strong>and</strong> for healthy products, the increasing<br />
legal restrictions on pesticides, along with the increase in resistance to pesticides, is<br />
driving the greenhouse industry to apply as many non-chemical solutions as possible,<br />
so that different kinds of control strategies have to interact (Hussey & Scopes, 1985;<br />
Tanigoshi, Martin, Osborne, & Peña, 2004; Gillespie & Raworth, 2004). In addition,<br />
during the last decade there has been a consistent <strong>and</strong> widespread increase in market of<br />
foodstuffs <strong>and</strong> other “biological” products. These are associated with natural <strong>and</strong><br />
healthy processes even if this association is frequently far from to be ascertained.<br />
Many countries, i.e. United Kingdom, have adopted strategies to reduce reliance on<br />
pesticides <strong>and</strong> encourage, or in some instances force, growers to consider other<br />
strategies in managing pests. This aim was pursued in 2006 <strong>by</strong> i.e. lowering<br />
registration fees associated with the development of biopesticides, in an effort to<br />
increase availability of reduced-risk pesticides to growers (ESRC, 2008).<br />
Campaigns against the use of pesticides in agriculture in the EU led to an increase<br />
of the production area <strong>and</strong> market size of the greenhouse industry, introducing<br />
biological control in many agricultural systems. Frequently <strong>and</strong> realistically, in spite of<br />
the great emphasis on the use of “natural” techniques concerning control <strong>and</strong><br />
production requiring the exclusion of artificial products, biological/<strong>org</strong>anic agriculture<br />
do not appear so different from most modern “conventional” regimes: these processes<br />
can be indeed largely based on the use of active ingredients, natural but still toxic that,<br />
on a different scale, could yield problems similar to those already known for pesticides<br />
(i.e. residues on foodstuffs, side effects on non-target <strong>org</strong>anisms).<br />
The global situation of pests control <strong>and</strong> the increasing efforts, both in biological<br />
<strong>and</strong> IPM agriculture, related to the adoptions of sustainable ways can be affected <strong>by</strong><br />
the lack of whole efficacy of these products, more than <strong>by</strong> a loss of strategic trust in<br />
pesticides. Given this context <strong>and</strong> perspectives, the control of pests matches frequently<br />
<strong>and</strong> unavoidably with the release <strong>and</strong>/or enforcing of natural enemies <strong>and</strong> antagonists<br />
already present on a crop (Bale, Van Lenteren, & Bigler, 2008).
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313<br />
Among natural enemies of arthropod pests, predaceous mites Phytoseiids<br />
(Acari: Mesostigmata), became in the recent years a fundamental tool for IPM in<br />
integrated crop production in Europe as well as worldwide. Various species or<br />
strains belonging to this group of predators are commonly used <strong>and</strong> marketed to<br />
control harmful insect <strong>and</strong> mite species. The phytoseiids ranking in different life<br />
style types, together with their quick adaptability to face new emergencies confirm<br />
their role as a significant <strong>and</strong> sustainable tool in biological control. In this chapter<br />
we review the basic concepts related to <strong>and</strong> the possible use of phytoseiids,<br />
including the enhancement <strong>and</strong> introduction of new strategies for efficient pest<br />
control, durable in time.<br />
2. CONCEPTS ON NATURAL ENEMIES AND/OR ANTAGONISTS IN IPM<br />
The role of natural enemies <strong>and</strong>/or antagonists in IPM <strong>and</strong> the degree at which<br />
biological control agents (BCAs) can be exploited vary from crop to crop <strong>and</strong> from<br />
area to area. Some questions need consideration <strong>and</strong> precise answers, before<br />
deciding on effectiveness of natural enemies against major pests on a crop system<br />
<strong>and</strong> defining the guidelines for their application or safeguard. One the most<br />
important issues concerns the occurrence of effective natural enemy on the<br />
considered pest <strong>and</strong> if, from an economic <strong>and</strong> ecologic point of view, it is more<br />
convenient to introduce mass reared enemies or to facilitate the colonization of the<br />
crop <strong>by</strong> local populations, from the surrounding areas. The crops or vegetation types<br />
adjacent to the targeted crop are important, since some plants can act as possible<br />
refuge for natural enemies, while others can harbour unwanted pests.<br />
Crops grown under "<strong>org</strong>anic" or "conventional" regimes obviously need<br />
different approaches for pest management. If the crop is "<strong>org</strong>anic" it can provide<br />
added incentives to the use of biocontrol methods. However, a crop does not have to<br />
be grown <strong>org</strong>anically to benefit <strong>by</strong> the use of biocontrol methods. "Soft" chemical<br />
options must be found for use in conjunction with natural enemies. Furthermore,<br />
crop life span <strong>and</strong> environment have to be suitable enough for harboring natural<br />
enemies. Generally, it can be difficult to establish BCAs in short lived crops. Also,<br />
the knowledge about plant life stages suitable for natural enemies is important, since<br />
BCAs may be most appropriate at a particular stage of the growing cycle.<br />
In addition to these questions, there are those related to the cost, practicality <strong>and</strong><br />
degree of difficulty encountered when controlling key pests with chemical means<br />
alone <strong>and</strong>/or natural enemies, <strong>and</strong> when assuming which strategy is more dem<strong>and</strong>ing<br />
in terms of cost, efficiency or healthy status returns. Furthermore, difficulties are<br />
encountered when switching from a conventional towards an IPM or <strong>org</strong>anic system.<br />
Practices <strong>and</strong> routines need to be modified continuously as new information must be<br />
gained during this process. Regular monitoring is necessary to identify pest<br />
outbreaks <strong>and</strong> their location within a crop. Also, "soft" controls methods should be<br />
checked <strong>and</strong> tested, since they may be available for some pests, but not for others.<br />
When an antagonists-based strategy is adopted, some damage induced <strong>by</strong> pests<br />
must be tolerated, since a minimum number of individuals may be required to<br />
support a useful population of its natural enemy. Deciding whether or not spraying
314<br />
S. SIMONI & M. CASTAGNOLI<br />
(<strong>and</strong> when) can represent a further difficulty. However, if "soft" options are<br />
available for the pest in question, this is not such an issue. The identification of the<br />
most appropriate release timing is necessary when introducing natural enemies <strong>and</strong><br />
to get them established quickly <strong>and</strong> maintained along. The introduction of<br />
appropriate numbers of mass reared BCAs is another condition necessary to<br />
facilitate quick establishment.<br />
Another aspect to be considered is providing a suitable environment. Very hot<br />
dry conditions are not conducive to some BCA's <strong>and</strong> research programs were<br />
recently developed (Palevsky et al., 2006). Adjustments may need to make to favour<br />
BCA's, e.g. shade, windbreaks, overhead watering. Having an expectation that one<br />
cannot spray chemicals at all could be incorrect <strong>and</strong> may result in failure of the IPM<br />
system. BCA's usually recover from occasional sprays of moderately toxic products<br />
<strong>and</strong> can remain at useful levels.<br />
Actually, <strong>by</strong> referring to the state of knowledge on animal <strong>org</strong>anisms <strong>and</strong> to the<br />
complex represented <strong>by</strong> phytophagous-natural <strong>and</strong>/or commercial enemies,<br />
consolidated strategies (<strong>and</strong> not only theoretical approaches) are available for<br />
farmers. They aim, among the several factors involved, to the reconstitution of the<br />
populations balance <strong>and</strong> to the improvement of the action against enemies. This<br />
objective is pursued <strong>by</strong>: (i) the diffusion of antagonists, (ii) the elimination of<br />
sources of perturbance <strong>and</strong> (iii) the adoption of environmental <strong>and</strong> cultural<br />
management measures.<br />
This chapter deals with the phytoseiid mites, which have a significant role on<br />
control of crop pests in greenhouse <strong>and</strong> field conditions, worldwide. By focusing on<br />
the definition of DeBach (1964), biological control is: the study <strong>and</strong> uses of<br />
parasites, predators <strong>and</strong> pathogens for the regulation of host (pest) densities. Two<br />
main principles are included in this review: (1) most <strong>org</strong>anisms are consumed <strong>by</strong><br />
other <strong>org</strong>anisms <strong>and</strong> this can be exploited <strong>by</strong> the man as “natural control”, (2) this<br />
natural/biological control reduces, rather than eradicates, the pest. As a consequence,<br />
a number of important pests can be kept at a low population density <strong>by</strong> biological<br />
control agents over long time periods or, differently, populations of pests are<br />
reduced but further releases, or additional methods are needed to achieve an<br />
adequate level of control. Among BCAs, phytoseiids are, for their traits, highly<br />
capable to efficiently interface with rapidly changing contexts, as crop <strong>and</strong><br />
environment turn over. At the same time, the great versatility of some species seems<br />
to guarantee long lasting control expectancy of pests <strong>and</strong> a presidium of the area<br />
with an acceptable level of related costs.<br />
3.1. Mass Rearing<br />
3. WHY PHYTOSEIIDS?<br />
The breeding of auxiliaries is a very complex task, requiring the development of<br />
refined <strong>and</strong> very reliable techniques. The high cost involved, together with the need<br />
to be supported <strong>by</strong> a sure market, has sometimes considerably limited the use of<br />
natural enemies. However, the environments to be protected usually hosts intensive<br />
or expensive cultures <strong>and</strong>, on the other h<strong>and</strong>, do not facilitate the dispersion of the
PREDATORY MITES IN IPM<br />
315<br />
antagonists. For this reason, processes optimising their efficacy <strong>and</strong> persistence are<br />
needed.<br />
A combination of control efficiency with low production costs <strong>and</strong> receptive<br />
markets is needed to support the development of effective mass rearing technologies<br />
for selected antagonists, including importation <strong>and</strong> cultures of appropriate natural<br />
enemies on alternative food, automated productions, testing of technologies for<br />
production <strong>and</strong> quality of predators, processing, storage, packaging, distribution <strong>and</strong><br />
release of natural enemies of insect <strong>and</strong>/or weed pests. Recently, more <strong>and</strong> more<br />
effective augmentative <strong>and</strong> classical biological control strategies for key pests have<br />
been developed.<br />
Phytoseiids satisfactorily match all the needs of the production pathway <strong>and</strong><br />
their production <strong>and</strong> marketing sensibly increased in the last years (Van Lenteren,<br />
2003). Some species i.e. Phytoseiulus persimilis <strong>and</strong> Neoseiulus californicus (Fig. 1)<br />
are worldwide employed in control strategies. They have been widely <strong>and</strong><br />
successfully used in the biological control of tetranychids phytophagous mites, for<br />
over half a century <strong>and</strong> more recently for thrips <strong>and</strong> aleurodids (Gerson &<br />
Weintraub, 2007; Messelink, Van Steenpaal, & Ramakers, 2006; Messelink,<br />
Maanen, Van Steenpaal, & Janssen, 2008). For many phytoseiids species the rearing<br />
can be conducted on a number of alternative preys, which lowered considerably the<br />
costs.<br />
Figure 1. Phytoseiulus persimilis preying on Tetranychus urticae on strawberry leaf (A), <strong>and</strong><br />
Neoseiulus californicus preying astigmatid mite on rearing unit (B).<br />
The large number of studies on biological traits of phytoseiids allowed<br />
producers to determine <strong>and</strong>/or automate the best mass rearing techniques <strong>and</strong> to<br />
establish their potential for control. At the same time research from bioindustries<br />
contributed to increase the bulk of knowledge, not only in terms of production<br />
st<strong>and</strong>ards <strong>and</strong>/or protocols to evaluate the quality <strong>and</strong> efficiency of reared predators,<br />
but also in terms of benefits for the theoretical study of predator-prey interactions.
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S. SIMONI & M. CASTAGNOLI<br />
3.2. Fitness <strong>and</strong> Adaptation Characters<br />
Phytoseiids have a short life span <strong>and</strong> are relatively easy to rear in the laboratory.<br />
For these reasons they are frequently chosen as a subject for basic studies on the<br />
mechanisms regulating the herbivores-predators-plants relationships. Some effective<br />
phytoseiids proved to retain high developmental <strong>and</strong> population increase rates on<br />
prey (Table 1), as well as good numerical <strong>and</strong> functional responses on prey density<br />
(Nachman, 1981; Sabelis, 1986; Castagnoli & Simoni, 1999). Data are available also<br />
on population dynamics <strong>and</strong> density changes in both seasonal <strong>and</strong> spatial<br />
distribution studies (Sabelis & Bakker, 1992; Sabelis & Janssen, 1994), as well as on<br />
mechanism <strong>and</strong> cues which determine the search of prey <strong>and</strong> infested plants (Sabelis<br />
& Van der Baan, 1983; Takabayashi, Dicke, & Posthumus, 1991). Data on the<br />
characteristics <strong>and</strong> occurrence of diapause <strong>and</strong> on the abiotic factors involved in its<br />
induction, maintenance <strong>and</strong> termination (i.e. photoperiod, temperature <strong>and</strong> food<br />
availability), are available for phytoseiid mites, as well as knowledge about the<br />
physiological mechanisms <strong>and</strong> related applied aspects (Veerman, 1992).<br />
Table 1. Intrinsic rate of increase (r m ) <strong>and</strong> population doubling time at about 25°C<br />
of phytoseiid species, largely utilized in biological control.<br />
Phytoseiid species<br />
Prey<br />
r m<br />
(day –1 )<br />
Doubling time<br />
(days)<br />
References<br />
Phytoseiulus<br />
persimilis<br />
Neoseiulus<br />
californicus<br />
Tetranychids 0.317 2.19<br />
Tetranychids 0.259 2.68<br />
Takafuji <strong>and</strong> Chant<br />
(1976)<br />
Castagnoli <strong>and</strong><br />
Simoni (1991)<br />
Neoseiulus cucumeris<br />
Tetranychids<br />
Thrips<br />
0.174<br />
0.178<br />
3.98<br />
3.89<br />
Castagnoli <strong>and</strong><br />
Simoni (1990)<br />
Amblyseius swirkii Whitefly 0.213 3.25<br />
Nomikou, Janssen,<br />
Schraag, <strong>and</strong> Sabelis<br />
(2001)<br />
Galendromus<br />
occidentalis<br />
Tetranychids 0.190 3.65<br />
Tanigoshi, Hoyt,<br />
Browne, <strong>and</strong> Logan<br />
(1975)<br />
However, the phytoseiids reproductive strategy is the trait which perhaps makes<br />
these predators quite peculiar. In arrhenotokous arthropods males arise from<br />
unfertilized eggs <strong>and</strong>, <strong>by</strong> controlling the fertilization process, mothers can adjust the<br />
sex ratio in their offspring. In pseudo-arrhenotokous phytoseiid mites, males are<br />
haploid, even if arising from fertilized eggs. The haploid state is achieved through<br />
elimination of a chromosome set during the embryonic development. Phytoseiid<br />
females can control the sex ratio in their offspring <strong>and</strong> this control seems extremely<br />
flexible (Nagelkerke & Sabelis, 1998). As predicted <strong>by</strong> current evolutionary theory
PREDATORY MITES IN IPM<br />
317<br />
of sex allocation, sex ratios approached half males, half females under r<strong>and</strong>om<br />
mating, whereas a female bias was observed under sib-mating. It is suggested that<br />
arrhenotoky is selected for when there is a substantial risk of high portion of<br />
unmated females in the population: pseudo-arrhenotoky may evolve <strong>by</strong><br />
external/environmental pressure, since it retains the possibility to reinstall lost genetic<br />
information in the maternally derived chromosome, <strong>by</strong> using the paternal chromosome<br />
as a template for DNA-repair. This precise control of sex allocation in phytoseiids is<br />
probably the significant mechanism <strong>by</strong> which these predators can regulate their<br />
density, depending on both phytoseiid female <strong>and</strong> prey densities. They can in fact<br />
adjust offspring sex ratio in response to the presence of conspecifics or their cues <strong>and</strong><br />
also to synchronize their population with that of prey (Nagelkerke & Sabelis, 1996).<br />
The prediction of optimal sex ratio <strong>by</strong> means of modeling is selectively advantageous<br />
when local mating groups vary in size <strong>and</strong> are usually small, as in the case of<br />
experimental laboratory studies on phytoseiids. At a larger spatial scale than the local<br />
mating group, the prediction appears to be less precise, may be due to operating <strong>and</strong><br />
interfering selection levels (Nagelkerke & Sabelis, 1998).<br />
3.3. Life Style Types<br />
The characterization <strong>and</strong> ranking of phytoseiid mites is a helpful <strong>and</strong> significant tool<br />
(McMurtry & Croft, 1997), allowing a rating of species based on some<br />
morphological, reproductive <strong>and</strong> developmental aspects. Furthermore, traits like<br />
feeding <strong>and</strong> diet needs (McMurtry & Rodriguez, 1987; Schausberger & Croft, 1999)<br />
<strong>and</strong> adaptation to certain foods (Castagnoli, Simoni, & Liguori, 2003), were<br />
considered to ascribe the predators to the different life styles. McMurtry <strong>and</strong> Croft<br />
(1997) considered that a four-types classification may be efficient to rank the<br />
different species of phytoseiids <strong>and</strong> gave emphasis to the biological control of spider<br />
mite pests (Table 2). However, new life style types might be identified.<br />
Recent studies aimed at estimating/identifying the more significant traits<br />
involved in phytoseiids rating <strong>and</strong> to possibly generate more stable classifications<br />
(Croft, Blackwood, & McMurtry, 2004). The mainly <strong>and</strong> first exploited traits/factors<br />
to rate phytoseiids were: (i) Feeding: the ability to prey <strong>and</strong> to feed on various prey<br />
<strong>and</strong> other food types (McMurtry & Rodriguez, 1987; McMurtry, 1992), a primary<br />
criterion considered for classification; (ii) External morphology: apparently, no<br />
strong correlation was found between body size <strong>and</strong> generalist–specialist phytoseiids<br />
(Schuster & Pritchard, 1963; Chant & Hansell, 1971) <strong>and</strong> more evidence is needed<br />
to establish the association between body size <strong>and</strong> different life styles (Croft et al.,<br />
2004); more correspondence was found in the evaluation of the adult dorsal shield<br />
setal length, in association with the feeding specialization (Sabelis & Bakker, 1992).<br />
Also, the mouthpart apparatus may be different between specialists <strong>and</strong> generalists<br />
(Flechtmann & McMurtry, 1992), but it is not clear to what extent this could work<br />
for a clear attribution to a life style; (iii) Biological parameters: research focused on<br />
reproduction, development <strong>and</strong> mortality; the specialist phytoseiids generally show<br />
intrinsic rates (Sabelis & Janssen, 1994) <strong>and</strong> sex ratio values higher than generalist<br />
(Nagelkerke & Sabelis, 1996) as well as shorter developmental times (Luh & Croft,
318<br />
S. SIMONI & M. CASTAGNOLI<br />
1999, 2001). Concerning mortality, studies characterized more exactly the<br />
dependence on prey density <strong>and</strong> the rate <strong>by</strong> which this changes. Through mortality,<br />
species differently adapt to varying prey or food levels, in the different life style<br />
types: the specialist species shows a tendence towards fast response to higher prey<br />
densities than a generalist, whereas a generalist tends to persist for a longer time, at<br />
limited or scarce prey density (Walzer & Schausberger, 2005; Simoni, Castagnoli, &<br />
Liguori, 2005).<br />
Table 2. Categorization of phytoseiids life style types <strong>by</strong> McMurtry <strong>and</strong> Croft (1997).<br />
Type Strategy a Crop b<br />
Type I spp.<br />
Phytoseiulus persimilis 1, 2, 3 L, G<br />
P. macropilis 2 L<br />
P. longipes 2 L, G<br />
Type II spp.<br />
Galendromus annectes 1, 2 T<br />
G. helveolus 1, 2 T<br />
G. occidentalis 1, 2, 3 T, L, V<br />
Typhlodromus (T.) rickeri<br />
T<br />
Neoseiulus bibens 1 L, Sh<br />
N. californicus 1, 2 T, L, V<br />
N. fallacis 1, 2, 3 T, Sh, L<br />
N. idaeus 1, 3 Sh, L<br />
N. longispinosus 1, 2 T, Sh, L<br />
N. tiki 1 Sh, L<br />
Type III spp.<br />
Typhlodromus (T.) pyri 1, 2 T, V, Sh<br />
T. (T.) exhilaratus 1 T<br />
T. (Anthoseius) caudiglans 1 T<br />
T. (A.) doreenae 1 V<br />
Metaseiulus arboreus 1 T<br />
M. citri 1 T<br />
M. pomi 1 T<br />
Paraseiulus soleiger 1 T
PREDATORY MITES IN IPM<br />
319<br />
Table 2 continued<br />
Type III spp. (continued)<br />
Phytoseius macropilis 1 T<br />
P. spoofi 1 T<br />
Amblyseius <strong>and</strong>ersoni 1, 2 T<br />
A. eharai 1 T<br />
A. swirskii 1 T<br />
Neoseiulus barkeri 2 G<br />
N. cucumeris 1, 2 L, G<br />
N. umbraticus L, T<br />
Kampimodromus aberrans 1,2 T, V<br />
Typhlodromalus aripo 1, 3 Sh<br />
T. limonicus 1 T, Sh<br />
T. manihoti 1, 3 Sh<br />
Typhlodromips sessor<br />
T. newsami 1, 2 T<br />
Iphiseius degenerans 1, 2 T, Sh, G<br />
Type IV spp.<br />
Euseius addoensis 1 T<br />
E. elinae 1 T<br />
E. finl<strong>and</strong>icus 1 T<br />
E. fructicolus 1 T<br />
E. sojaensis 1 T<br />
E. tularensis 1 T<br />
E. stipulatus 1,3 T<br />
E. victoriensis 1 T<br />
a Strategies: 1 = conservation; 2 = augmentation; 3 = importation <strong>and</strong> establishment.<br />
b Crops: L = low-growing; G = greenhouse; T = tree; Sh = shrub; V = grapevine.<br />
A considerable amount of studies has been recently added concerning the<br />
evaluation of the different degree of responses <strong>by</strong> generalists <strong>and</strong> specialists<br />
predators, as a consequence of their different physiology <strong>and</strong> behaviour. Even if a<br />
build up in basic physiological studies is still necessary, physiological <strong>and</strong><br />
behavioural responses were analysed frequently <strong>and</strong> in different contexts.<br />
Preliminary studies indicate appreciable differences among life styles. One of the<br />
most remarkable concerns the response to odours produced <strong>by</strong> preys, other foods,<br />
competitors, host plants <strong>and</strong> other habitat-related elements (Blackwood, Luh, &<br />
T
320<br />
S. SIMONI & M. CASTAGNOLI<br />
Croft 2004; Gnanvossou, Hanna, & Dicke, 2003; Schausberger & Croft, 2001). In<br />
particular, host–plant relationships seem to be especially affected <strong>by</strong> the intrinsic<br />
physiological traits, <strong>and</strong> generalists have closer associations with host plants than<br />
specialist phytoseiids do (Kreiter, Tixier, Croft, Auger, & Barret, 2002; Tixier,<br />
Kreiter, Croft, & Auger, 2002). Specialists also tend to aggregate mostly in<br />
proximity of preys, <strong>by</strong> suffering sometimes higher mortalities (McMurtry & Croft,<br />
1997; Faraji, Janssen, & Sabelis, 2002), whereas the perception of the prey cues can<br />
lead to different inter <strong>and</strong>/or within plant dispersal.<br />
It should be considered that the phytoseiids life style categorization is not a<br />
dogma, although it can be represent a dynamic underlying support in setting control<br />
strategies of different pests. To determine the value of each definition, a sort of<br />
holistic approach would be advisable, <strong>by</strong> considering more factors <strong>and</strong> criteria in the<br />
grouping. Future studies are needed to estimate both the optimal numbers of traits<br />
<strong>and</strong> numbers of life styles type, simultaneously. Such fitting problems, or more<br />
robust classifications, probably will require the use of a multi-sample classification<br />
methods. By this point of view, significant trials were performed <strong>by</strong> Luh <strong>and</strong> Croft<br />
(1999, 2001) <strong>by</strong> a computer-based genetic algorithm, <strong>and</strong> <strong>by</strong> Blackwood et al.<br />
(2004), <strong>by</strong> a discriminant analysis model. The results obtained <strong>by</strong> Luh <strong>and</strong> Croft<br />
(2001) were in full agreement with the ranking of McMurtry <strong>and</strong> Croft (1997): just<br />
one, Neoseiulus longispinosus, out the 20 species considered in the two<br />
categorizations shifted <strong>by</strong> one style type level. The selection of subsets of variables<br />
optimizing the classification <strong>and</strong> reducing the chance of misclassification of traits<br />
included for best fit, shows to be effective as identifying potential useful indicators<br />
of life style type.<br />
3.4. Single or Multiple Antagonists Release<br />
Several herbivores can be usually attacked <strong>by</strong> numerous predator species but,<br />
historically, studies concerning single prey-single predator interactions were mainly<br />
performed (Holling, 1966; Hassell, 1978; Kareiva, 1994). A controversial issue was<br />
the use of a natural enemy complex, as opposed to a single enemy strategy, to<br />
achieve the best biological control (Ehler, 1990; Riechert & Lawrence, 1997; Losey<br />
& Denno, 1998). As concerns mite pests management, control in different<br />
agricultural systems was generally performed <strong>by</strong> adopting the release of a single<br />
phytoseiid species. More sporadic were evaluations about the release of two or more<br />
species. The interaction <strong>and</strong> dynamics of different phytoseiids spp. with, evenly,<br />
different life styles, may return different responses in comparison with the expected<br />
outcome (Helle & Sabelis, 1985; McMurtry & Croft, 1997; Schausberger & Walzer,<br />
2001; Castagnoli, Simoni, & Nachman, 2001).<br />
Walzer <strong>and</strong> Schausberger (2005) evidenced that the combination of a specialist<br />
predator as Phytoseiulus persimilis <strong>and</strong> a diet-generalist as Neoseiulus californicus<br />
in a sustainable way, might control spider mite, with higher efficiency in perennial<br />
crops. Control on eggplant <strong>and</strong> pepper was achieved <strong>by</strong> single N. californicus<br />
release (Castagnoli, Liguori, & Simoni, 2005). Simoni et al. (2005) evaluated the<br />
same phytoseiids <strong>and</strong> P. persimilis alone, <strong>by</strong> means of single <strong>and</strong> combined releases,<br />
on the same infested solanaceae as well as on tomato, in order to evaluate if their
PREDATORY MITES IN IPM<br />
321<br />
effect was additive, multiplicative or detrimental in the action of predators. The notoverlapping<br />
degree of specialization, narrow in P. persimilis, wider in N.<br />
californicus, <strong>and</strong> the consequent asymmetry in the response guaranteed, for some<br />
weeks, fast (mainly due to P. persimilis) <strong>and</strong> longer (mainly due to N. californicus)<br />
term equilibrium of the prey-predator system <strong>and</strong> of biological control, especially on<br />
eggplant <strong>and</strong> pepper.<br />
As concerns the ascertained intrinsic traits <strong>and</strong> versatility of some phytoseiid, N.<br />
californicus appears able to adapt to different food <strong>and</strong> climatic conditions<br />
(Castagnoli & Simoni, 2004), <strong>and</strong> it may be considered feasible <strong>and</strong> convenient if<br />
combined to or in light shifts of phytoseiid releases, or in application with some<br />
other kind of biocontrol agents (i.e. other mites, insects or the fungus Beauveria<br />
bassiana). Obviously, the adoption of such a tactic needs an intensive monitoring, a<br />
full evaluation of the possible effect of the micr<strong>org</strong>anism on the predator <strong>and</strong> an<br />
assessment concerning the possibility that the phytoseiid is able to recognize the<br />
treated substrate (Simoni, Guidi, & Tarchi, 2009).<br />
3.5. Cannibalism <strong>and</strong> Intraguild Predation<br />
The coexistence <strong>and</strong> interaction of two different phytoseiids species sharing a<br />
common prey resource can undoubtedly determine new functional-trophic relations<br />
(Rudolf, 2008). Intraguild predation <strong>and</strong> cannibalism are, in cases of combined<br />
release of predators, variables to be included in current models aiming at<br />
overcoming the discrepancy between theory <strong>and</strong> empirical data.<br />
Although cannibalism may often represent a weak, unuseful interaction in<br />
nature, it may have significant consequences at the population level (McCann,<br />
Hastings, & Huxel, 1998). Cannibalism can be a crucial factor contributing to<br />
population structure, dynamics <strong>and</strong> control in a given habitat (McCann et al., 1998),<br />
affecting the quantity <strong>and</strong> quality of food for the remaining individuals. Predatorpredator<br />
interactions such as competition, intraguild predation (IGP), <strong>and</strong><br />
cannibalism affect the development <strong>and</strong> coexistence of predator populations, <strong>and</strong><br />
can have significance in the biological control of commonly exploited pest<br />
<strong>org</strong>anisms (Castagnoli, Liguori, & Simoni, 2002; Schausberger & Croft, 2000).<br />
Furthermore, phytoseiids are suitable models for studying cannibalism <strong>and</strong> related<br />
phenomena, due to their diversity <strong>and</strong> variability, small size <strong>and</strong> ease of rearing in<br />
the laboratory. In future research <strong>and</strong> in the frame of tactics <strong>and</strong> strategies of control,<br />
most fields are to be exploited, i.e. kin the link of cannibalism with discrimination<br />
<strong>and</strong> disease transmission, the interplay between cannibalism <strong>and</strong> dispersal, <strong>and</strong> the<br />
effects of cannibalism on population dynamics <strong>and</strong> species communities.<br />
4. CONCLUSIONS<br />
Given the number <strong>and</strong> complexity of factors involved in the wide pattern of natural<br />
enemies <strong>and</strong> antagonists, phytoseiid mites appear able to significantly interact in the<br />
dynamic equilibria of different prey-crop contexts. The modality of agricultural<br />
pests control <strong>by</strong> these predators can range from classical biological control, with<br />
introduction <strong>and</strong> establishment of foreign species, to safeguard <strong>and</strong> augmentation of
322<br />
S. SIMONI & M. CASTAGNOLI<br />
indigenous species. Perspectively, it appears convenient to stress further the search<br />
for appropriate control strategies <strong>and</strong> tactics, on which phytoseiids have a dominant<br />
role. Phytoseiids proved to be able to quickly adapt to new environmental conditions<br />
(Helle & Sabelis, 1985). Laboratory selection of phytoseiids produced several<br />
strains with different traits as no-diapausing strains, strains adapted to live on<br />
unsuitable hosts or more resistant to adverse climate or pesticides (Castagnoli,<br />
Liguori, Simoni, & Guidi, 1998; Castagnoli, Liguori, & Simoni, 1999; Castagnoli<br />
et al., 2003; Drukker, Janssen, Ravensberg, & Sabelis, 1997; Fournier, Pralavorio,<br />
Berge, & Cuany, 1985). Frequently, these adapted strains have been mass reared <strong>and</strong><br />
released for pest management programs in glasshouses <strong>and</strong> agricultural cropping<br />
systems. The majority of researches on the argument show that the release of<br />
phytoseiids for augmentation or classical biological control programs involves<br />
minimal risk for the environment <strong>and</strong> indigenous predators, with great benefits<br />
(Pilkington, Messelink, Van Lenteren, & Le Mottee, 2009).<br />
The development of recombinant DNA techniques for the genetic manipulation<br />
of crops <strong>and</strong> micro<strong>org</strong>anisms may be successfully applied also to phytoseiids, <strong>and</strong><br />
much debated opinions concern risks of transgenic phytoseiids release. Great<br />
attention <strong>and</strong> punctual researches still need to address the real impact in the<br />
environment of phytoseiids that have been manipulated with genetic techniques.<br />
These studies, further to answer to the question, could again provide opportunities to<br />
exp<strong>and</strong> our underst<strong>and</strong>ing of the ecological impact of phytoseiids in agricultural <strong>and</strong><br />
natural environments, <strong>and</strong> lead to improved pest management tactics (Hoy, 1992).<br />
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α-copaene, 92<br />
α Proteobacteria, 257<br />
α-ylangene, 92<br />
β-exotoxin, 254<br />
δ-endotoxin, 254, 255<br />
(1R-CIS)-3-isopropenyl-2.2-<br />
dimethylcyclobutyl-methyl acetate,<br />
14<br />
(3Z, 6R)-3-methyl-6-isopropenyl-3.9-<br />
decadien-l-yl acetate, 14<br />
1,4 diaminobutane, 32<br />
16S rDNA, 255, 258, 296<br />
18S ribosomal DNA, 268<br />
18S, 118<br />
4,8-dimethylnona-1, 3, 3-triene, 200<br />
4-methyl-5-nonanol, 218<br />
4-methyl-5-nonanone, 218<br />
5.8S, 118<br />
5.8S rRNA gene, 118<br />
A<br />
Abacarus hystrix, 265, 274, 275<br />
Abamectin, 21, 24, 25, 44, 68<br />
ABC, 17, 19<br />
Abdomen, 75, 87, 89<br />
Abdominal segments, 80<br />
Abundance, 107, 109, 111, 112, 113,<br />
115, 123, 137, 140, 195, 199, 204<br />
Acacia, 76, 79<br />
Acalitus vaccinii, 275<br />
Acalyptris minimella, 83<br />
Acarapis woodi, 253<br />
Acari, 61, 66, 67–68, 77, 249, 250,<br />
273, 295, 299–300<br />
Acaricidal preparations, 299<br />
Acaricides, 5, 21, 23, 51, 53, 251, 254,<br />
255, 278, 279, 283, 285, 297, 299<br />
Acaridae, 264, 274, 280, 287, 288<br />
Acariformes, 11<br />
Acariformis phytoseiuli, 300<br />
Acarofauna, 69<br />
Acarogregarina corolla, 287<br />
Acaromyces ingoldii, 285<br />
Accidental introduction, 74<br />
INDEX<br />
Accuracy, 117, 119<br />
Aceratoneuromyia indica<br />
(= Syntomosphyrum indicum), 20<br />
Aceria (Eriophyes) guerreronis, 278<br />
Aceria cynodoniensis, 275<br />
Aceria guerreronis, 275, 279<br />
Aceria sheldoni, 29, 30, 50, 51, 275<br />
Aceria tulipae, 252, 306<br />
Aceria vaccinii, 283<br />
Aceria, 252, 275, 278, 283, 306, 308<br />
Acetamiprid, 21–24, 45, 68<br />
Acetosphora, 289<br />
Acetylated derivatives, 200, 208<br />
Achaia, 30, 31, 48<br />
Acrididae, 7<br />
Acrinathrin, 21, 23, 24<br />
Acrobasis nuxvorella, 138<br />
Acrosternum hilare, 155<br />
Active compounds, 22<br />
Active ingredient, 22–24, 26, 66–68,<br />
279, 299<br />
Active substances, 35, 39, 41, 44, 47,<br />
49, 50, 53<br />
Activity, 214, 233<br />
Aculodes, 265<br />
Aculops lycopersici, 275<br />
Aculops pelekassi, 11, 29, 30, 50, 51<br />
Aculus fockeui, 265<br />
Adalia bipunctata, 46<br />
Adalia decempunctata, 46<br />
Adaptation, 190, 192, 196, 205<br />
Adelina acarinae, 288<br />
Adhesive knobs, 115<br />
Administrative boundaries, 165<br />
Adulticides, 104<br />
Adults, 13, 14<br />
Aegina, 31<br />
Aerial control, 240<br />
Aerial platforms, 167, 172<br />
Aerial treatment, 240–241<br />
Afghanistan, 83<br />
Aflatoxin, 284<br />
Africa, 83, 87, 89, 164, 165, 170,<br />
172, 173, 181, 182, 184, 185, 187,<br />
327<br />
A. <strong>Ciancio</strong>, K.G. Mukerji (eds.), Integrated Management of Arthropod Pests<br />
<strong>and</strong> Insect Borne Diseases, Integrated Management of Plant Pests <strong>and</strong> Diseases 5,<br />
DOI 10.1007/978-90-481-8606-8, © Springer Science+Business Media B.V. 2010
328<br />
INDEX<br />
237, 238, 241, 268, 269, 271, 280,<br />
298, 305, 309<br />
African citrus psylla, 6<br />
Aganaspis (Trybliographa) daci, 34<br />
Ageniaspis citricola, 43, 54, 63, 81,<br />
82<br />
Aggregation Pheromone Traps, 209,<br />
218, 223, 231<br />
Aggregation pheromone, 209, 211,<br />
218, 219, 222, 223, 231–233<br />
Agistemus, 264<br />
Agricultural systems, 312, 320<br />
Agriculture, 22<br />
Agrobacterium tumefaciens, 137, 141<br />
Agrochemicals, 5<br />
Agroecosystem, 47, 312, 324<br />
Agromyza hiemalis, 84, 97<br />
Agromyzidae, 84, 97<br />
Agronomic management, 94<br />
Agronomist, 31<br />
Air currents, 236<br />
Airways, 236<br />
Alaskozetes antarcticus, 265, 268, 301<br />
Albendazole, 294<br />
Alder, 76<br />
Aleurocanthus spiniferus, 74, 98<br />
Aleurocanthus woglumi, 74<br />
Aleuroclava jasmini, 74<br />
Aleurodicus dispersus, 74<br />
Aleurothrixus floccosus, 8, 23, 29–31,<br />
40–42, 55, 57, 62–64, 74, 93, 97, 98<br />
Aleyrodidae, 8, 23, 29, 30, 40, 41,<br />
54–58, 63, 64<br />
Alfamethrin, 21<br />
Algae, 286<br />
Algeria, 4, 82<br />
Alimentary tract, 250, 252, 253, 254<br />
Allergenic structures, 236<br />
Allium canadense, 196<br />
Allium, 252<br />
Alloxysta, 46<br />
Almond, 76<br />
Alnus rubra, 193, 208<br />
ALOS, 168<br />
alpha-cypermethrin, 21, 23, 24<br />
Alternate prey, 153<br />
Alternative host plants, 140<br />
Alternative hosts, 61, 67, 84, 86<br />
Alternative prey, 68<br />
Aluminum phosphide, 217, 218<br />
Amaranthus, 143<br />
Amblyseius <strong>and</strong>ersoni, 51, 319<br />
Amblyseius barkeri, 299<br />
Amblyseius cucumeris, 299<br />
Amblyseius eharai, 319<br />
Amblyseius igarassuensis, 264<br />
Amblyseius swirskii, 319<br />
Amblyseius, 264, 276, 288, 292, 300,<br />
308<br />
America, 135, 159, 160, 162<br />
Ameronothridae, 265, 268<br />
Amitus spiniferus, 63, 93<br />
AML, 177<br />
Ammonia, 35<br />
Ammonium acetate, 32<br />
Ammonium, 92<br />
Amoebae, 286<br />
Amoebozoa, 286<br />
Amrineus cocofolius, 274<br />
Amsterdam, 249, 300, 303, 305, 308<br />
Amudarya River, 178, 186, 187<br />
Anacridium aegyptium, 7<br />
Anagyrus pseudococci, 38, 65, 66,<br />
71, 87, 88<br />
Anal atrium, 294<br />
Anal tuft, 239<br />
Anaphe p<strong>and</strong>a, 239<br />
Anaphe, 239, 244<br />
Anaphylactic reactions, 236<br />
Ancylistaceae, 261, 262<br />
Angelica archangelica, 92<br />
Animal manure, 106, 111, 114<br />
Animals, 237, 239<br />
Anisolabis maritima, 215<br />
Annual broadleaf weeds, 146<br />
Anoplophora chinensis, 74<br />
Antarctica, 163<br />
Antennae, 80, 87<br />
Anthelidae, 236<br />
Anthracnose, 141<br />
Antibiotics, 259, 296<br />
Antidesiccants, 228, 232
INDEX<br />
329<br />
Ants, 13, 46, 47, 78, 81, 87, 88, 93,<br />
95, 96<br />
Aonidiella aurantii, 6, 9, 14, 23, 29–31,<br />
36, 37, 39, 63, 65, 74–76, 78, 94,<br />
97, 99, 100<br />
Aonidiella citrina, 74<br />
Apex, 50, 75, 262<br />
Aphelinidae, 37, 40, 54, 55, 58, 77,<br />
79, 93, 97, 98, 99<br />
Aphid colonies, 47<br />
Aphid parasitoids, 69<br />
Aphid populations, 69, 153, 154, 155<br />
Aphid predators, 46<br />
Aphid species, 139, 162<br />
Aphid vector, 94<br />
Aphid, 14, 53<br />
Aphidae, 67<br />
Aphidicides, 139<br />
Aphididae, 8, 23<br />
Aphidius colemani, 69<br />
Aphidius matricariae, 46<br />
Aphidius urticae, 46<br />
Aphidophaga, 153, 154, 157<br />
Aphidophagous coccinellid, 46<br />
Aphidophagous insects, 48, 133, 154<br />
Aphids, 13, 14, 22, 23, 29–31, 42,<br />
45–48, 53, 55, 68, 69, 134, 139,<br />
140, 142, 148, 152, 153, 154, 156,<br />
157, 159, 161, 193, 194, 200<br />
Aphis craccivora, 8, 45<br />
Aphis fabae, 8<br />
Aphis gossypii, 8, 23, 29, 45, 56, 62,<br />
63, 65, 67, 75, 94, 99<br />
Aphis nerii, 67<br />
Aphis spiraecola, 8, 23, 29, 45, 65,<br />
67, 74, 94<br />
Aphytis chilensis, 38<br />
Aphytis chrysomphali, 38, 77<br />
Aphytis coheni, 37<br />
Aphytis lepidosaphes, 30, 37, 63<br />
Aphytis lingnanensis, 37, 63, 77<br />
Aphytis melinus, 37, 63, 65, 77, 78,<br />
97, 98, 99, 100<br />
Aphytis proclia, 77<br />
Aphytis yanonensis, 10<br />
Apical twigs, 13<br />
Apicomplexa, 286, 287, 289<br />
Apis mellifera, 253<br />
Apotetrastichus postmarginalis, 86<br />
Apotetrastichus sericothorax, 86<br />
Apples, 31<br />
Application threshold, 36<br />
Application, 35, 50, 51, 226, 233,<br />
249, 250, 273, 279, 281, 283, 284,<br />
297, 299, 308<br />
Aprostocetus, 86<br />
Aqueous suspension, 251<br />
Arabidopsis thaliana, 200, 202<br />
Arabidopsis, 197, 198, 207, 208<br />
Arachnida, 70<br />
Aralia, 76<br />
Araneae, 70<br />
Araucaria, 76<br />
Arbutus unedo, 238<br />
Archery equipment, 134<br />
Archips rosanus, 10, 75, 94<br />
Arctiidae, 134, 236<br />
Arctoseiinae, 264<br />
Arctoseius, 264<br />
Argentina, 82, 278, 299, 307<br />
Argentine ants, 154, 161<br />
Argolis, 30, 31, 42, 43, 54<br />
Arizona, 135, 251, 297<br />
Armoured scale, 14, 37, 38, 75, 94, 99<br />
Arrhenotokous, 50, 259<br />
Arrhenotoky, 317<br />
Arrowleaf sida, 143<br />
Artemisia, 181<br />
Arthrobacter globiformis, 256<br />
Arthrobotrys oligospora, 115<br />
Arthropod densities, 151<br />
Arthropod hosts, 257<br />
Arthropod pest, 23, 29–31, 73, 313<br />
Arthropoda, 261<br />
Arthropodofauna, 69<br />
Arthropods, 6, 53, 67, 106, 112, 123,<br />
125, 126, 236, 246, 259–262, 277,<br />
286, 289<br />
Artificial habitat, 116<br />
Artificial media, 264, 270, 278, 295,<br />
297<br />
Artificially wounded leaves, 191, 200
330<br />
INDEX<br />
Asaphes vulgaris, 46<br />
Asaphes, 46<br />
Asca, 264<br />
Asci, 260, 286<br />
Ascidae, 275<br />
Ascomycota, 260, 272, 285<br />
Ascospores, 260, 286<br />
Asecodes delucchii, 86<br />
Asian Citrus Psyllid, 102<br />
Asparagus, 79<br />
Aspergillus flavus, 284, 307<br />
Aspergillus, 284, 296, 307<br />
Aspidiotus nerii, 9, 23, 39, 68, 74, 79<br />
Asterophora caloglyphi, 287<br />
Astigmatid mite, 315<br />
Astipalea, 42<br />
Asynonychus godmani, 11<br />
ATP synthase-subunit, 199<br />
Attack, 79, 81, 212, 235, 237, 240<br />
Attica, 31, 42, 44, 47, 58<br />
Attractants, 14, 21–23, 92<br />
Augmentation, 40, 55, 62, 101–103,<br />
105, 106, 111, 124, 129<br />
Augmentative biological control, 3,<br />
7, 21, 70<br />
Augmentative release, 53<br />
Aulacorthum solani, 8, 45<br />
Australasia, 64<br />
Australia, 43, 54, 57, 64, 66, 72, 82,<br />
83, 84, 89, 92, 96, 98, 170, 172,<br />
179–184, 239, 243, 244<br />
Australian plague locust, 179, 180,<br />
182, 184<br />
Authorization, 22<br />
Autogenous defensive secretions, 196<br />
Autumn, 13, 14, 104, 241, 267<br />
Avocado, 76<br />
Azadirachtin, 21–25, 41, 44, 47, 68<br />
Azobacter, 150<br />
Azocyclotin, 53<br />
Azores, 6, 12<br />
B<br />
Bacillus sphaericus, 256<br />
Bacillus thurigiensis var. aizawai, 21,<br />
22, 24, 49<br />
Bacillus thuringiensis var. kurstaki,<br />
21, 22, 24, 49, 240<br />
Bacillus thuringiensis, 67, 68, 107,<br />
134, 235, 236, 243–244, 254–256,<br />
299, 301, 303–304, 306<br />
Bacteria symbiosis, 123<br />
Bacteria, 105, 112, 116, 119, 123,<br />
147, 150, 151, 157, 209, 249, 255,<br />
259–260, 295, 300, 302<br />
Bacterial cells, 216<br />
Bacterial disease, 102<br />
Bacterial leaf scorch, 141<br />
Bacterial spores, 243<br />
Bacterium, 102, 113, 215, 235, 236,<br />
254, 255, 258, 259, 296, 300<br />
Bacteroidetes, 256, 259<br />
Bactrocera oleae, 35<br />
Baculoviruses, 295<br />
Baermann funnel, 121, 122<br />
Bahamas, 82<br />
Bahiagrass, 143, 146<br />
Bahrain, 209, 232<br />
Bait spraying, 34<br />
Balkans, 89<br />
Ballistospores, 261<br />
Banker plants, 67<br />
Baryscapus, 86<br />
Baseball bats, 134<br />
Basidiobolus, 264<br />
Basidiomycota, 260, 261, 272, 285<br />
Basque Country, 6<br />
Basudin, 217<br />
BC programs, 61, 64, 65<br />
BCAs, 313, 314<br />
Beauveria bassiana, 21, 22, 24, 216,<br />
231, 283, 284, 299, 321, 325<br />
Beauveria brongniartii, 283<br />
Beauveria, 283, 296, 299, 300, 305,<br />
307<br />
Bee Kashmir Virus, 253<br />
Bee, 148, 253, 284, 297, 302, 304,<br />
305, 307<br />
Beet army worm, 199, 201<br />
Beetle, 211, 232<br />
Behavior, 255, 300<br />
Beijing-1, 168
INDEX<br />
331<br />
Belgium, 175<br />
Belt, 240<br />
Bemisia hancocki, 8<br />
Bemisia tabaci, 8<br />
Beneficial arthropods, 5, 21, 25, 151,<br />
280<br />
Beneficial insects, 133, 139, 148<br />
Beneficial mites, 133, 249<br />
Beneficial <strong>org</strong>anisms, 26, 102<br />
Benfuracarb, 21, 23–25, 68<br />
Benin, 271, 281, 298, 309<br />
Bergamot, 4, 22, 29, 73<br />
Bermudagrass, 143<br />
Bifentrin, 21, 23, 24, 25<br />
Big bud disease, 283<br />
Bigarade orange, 3<br />
Binodoxys acalephae, 46<br />
Binodoxys angelicae, 46<br />
Bioactivity, 218<br />
Biocides, 240<br />
Biocontrol agent, 215, 230<br />
Biocontrol methods, 313<br />
Biocontrol, 101, 103, 107, 110, 114<br />
Biodiversity, 192<br />
Bio-ecological equilibrium, 73<br />
Bioindustries, 315<br />
Biological control agents, 36, 235,<br />
236, 249, 251, 256, 285, 292, 298,<br />
299, 303, 308, 314<br />
Biological control programs, 74, 78,<br />
81, 89, 92, 93<br />
Biological control, 3, 6, 7, 21, 26, 27,<br />
33, 36–38, 40–43, 45–48, 51, 53,<br />
54–55, 58, 64, 70, 71, 74, 77, 78,<br />
82, 85–88, 92–96, 100–103, 106,<br />
110, 111, 113, 120, 123, 124–129,<br />
134, 139, 152, 154, 204, 205, 218,<br />
224, 231–233, 249–252, 255,<br />
269–271, 278, 283, 285, 292, 295,<br />
298, 299, 301, 302, 307–308,<br />
311–317, 320, 321, 323, 324<br />
Biological parameters, 260, 317<br />
Biomass consumption, 192<br />
Biomass transfer, 203<br />
Biopesticide, 106, 123, 240, 241, 243<br />
Biorational insecticides, 138<br />
Biosynthetic pathways, 200<br />
Biotechnical methods, 34<br />
Biotic environment, 203<br />
Bird peck damage, 134<br />
Bird, 134, 135, 151, 157, 160<br />
Birefringent bodies, 251<br />
Birefringent crystals, 252, 293, 294<br />
Bitter orange, 29, 34, 36, 39, 45<br />
Black pecan aphid, 136, 138, 139,<br />
153<br />
Blackmargined aphid, 138, 139<br />
Blastic conidiogenesis, 296<br />
Blue lupine, 148<br />
Blueberry mites, 283<br />
Body cavity, 263, 284, 290<br />
Bohemia, 268<br />
Bombix mori, 197<br />
Bom<strong>by</strong>cidae, 236<br />
Borax, 32, 33<br />
Borers, 64<br />
Botanical pesticides, 278<br />
Bougainvillea, 76<br />
Bovine serum albumin, 120<br />
Boxwood, 76<br />
Brachycaudus helichrysi, 45<br />
Braconidae, 16, 20, 64, 65, 81, 92<br />
Bradysia impatiens, 198<br />
Branches, 14, 76, 79, 87, 88, 93, 237,<br />
284<br />
Brassica napus, 197, 207<br />
Brazil, 82, 168, 252, 267–271, 278,<br />
279, 281, 282, 283, 284, 298, 300,<br />
302–330, 307, 308<br />
Breeding programs, 143<br />
Breeding, 173, 179, 186<br />
Brevipalpus californicus, 12, 259<br />
Brevipalpus phoenicis, 12<br />
Bristles, 286<br />
Broad spectrum insecticides, 42, 138,<br />
139<br />
Brome Mosaic Virus, 252<br />
Brown citrus aphid, 6, 74<br />
Brown stink bug, 155<br />
Brown Tail Moth, 241<br />
Bryobia praetiosa, 258<br />
Bryobia, 256, 264, 266, 267
332<br />
INDEX<br />
Btk spore, 243<br />
Btk, 240–243<br />
BTM, 241<br />
Bugs, 81<br />
Bulb, 68<br />
Buprofezin, 21–25, 68, 77, 79, 89<br />
Bursaphelenchus mucronatus, 130<br />
Bursaphelenchus xylophilus, 130<br />
Buzzing, 214<br />
C<br />
Cabbage white butterfly, 196<br />
Cabinetry, 134<br />
Cacoecimorpha pronubana, 10<br />
Cadavers, 250, 273, 282, 285<br />
Calabria, 82<br />
Calacarus heveae, 275, 281–282, 308<br />
Calcium polysulfur, 21<br />
Calcium, 200<br />
Cales noacki, 15, 25, 40, 54, 63, 64,<br />
67, 68, 93, 94<br />
California red scale, 6, 29, 30, 36, 37,<br />
39, 74, 75, 77, 78, 95, 96, 98, 99<br />
California, 64, 66, 72, 74, 75, 77, 78,<br />
89, 94, 95–99, 104, 125, 135, 157,<br />
250, 251, 253, 297, 308<br />
Calliptamus italicus, 181, 187<br />
Calocoris trivialis, 7, 13, 75<br />
Caloglyphus moniezi, 287<br />
Calyx, 50<br />
Cambium layer, 134<br />
Camellia, 76<br />
Cameras, 166<br />
Camponotus nyl<strong>and</strong>eri, 11, 89<br />
Campsis radicans, 143<br />
Canada, 240<br />
Canary Isl<strong>and</strong>s, 6, 19, 20, 63, 64<br />
C<strong>and</strong>elilla wax powder, 284<br />
C<strong>and</strong>idatus Liberibacter asiaticus,<br />
102<br />
C<strong>and</strong>idatus Liberobacter, 6<br />
Cannibalism, 294, 321, 322, 323, 324<br />
Cannon, 262<br />
Canopy, 14, 104, 108, 116, 134, 154<br />
Capilliconidia, 269, 270, 306<br />
Capilliconidium, 263, 296<br />
Capture, 77, 78, 88, 219–223, 229<br />
Carabodes coriaceus, 287, 289<br />
Carabodes femoralis, 289<br />
Carabodidae, 287, 289<br />
Carbaryl, 138, 158, 216<br />
Carbofuran, 218<br />
Carbosulfan, 21, 23–25<br />
Cardinium, 257, 259, 300, 302, 303<br />
Carfentrazone, 144<br />
Caribbean, 104, 110, 125<br />
Carnauba, 284<br />
Carob, 76, 79<br />
Carya illinoinensis, 133, 159<br />
Cassava belt, 269, 280<br />
Cassava green mite, 262, 268–271,<br />
280, 298, 302–303, 306, 309<br />
Cassava mites, 298<br />
Cassava, 262, 268–271, 280, 298,<br />
300, 302–303, 306, 309<br />
Caterpillar, 134, 191, 196, 197, 201,<br />
206<br />
Caterpillars dieting, 197<br />
CBC, 15–20<br />
CBERS-2, 168<br />
Cecidomyidae, 77<br />
Cecidomyids, 67<br />
Cecidophyes galii, 283<br />
Cecidophyopsis ribis, 283<br />
Cecropia insignis, 194<br />
Cecropia, 194<br />
Cedrus, 237<br />
Cells, 251, 252, 253, 255, 258, 261,<br />
272, 285, 286, 290, 291, 292, 293,<br />
304<br />
Celphos, 217<br />
Cement, 217<br />
Central America, 88, 89<br />
Central Asia, 177, 181, 185<br />
Cephalosporium, 296, 300<br />
Cepheoidea, 289<br />
Cepheus dentatus, 289<br />
Ceratitis capitata, 6, 11, 13, 14, 20,<br />
24, 31–33, 34–35, 55, 57–59,<br />
62–64, 69, 72, 74–75, 89–92, 95<br />
Ceratoppia bipilis, 288<br />
Ceratoppia, 288
INDEX<br />
333<br />
Ceratozetidae, 287<br />
Cereal crops, 179<br />
Ceroplastes floridensis, 9, 38, 74<br />
Ceroplastes japonicus, 9<br />
Ceroplastes rusci, 9, 29, 30, 31, 36,<br />
38, 75, 94<br />
Ceroplastes sinensis, 9, 23, 62<br />
Certification, 5<br />
Cetonia carthami, 11<br />
CGM, 269, 270, 271, 281<br />
Chaff scale, 75<br />
Chalcididae, 20<br />
Chania, 43, 47, 49, 50, 54, 57, 59<br />
Charaxes jasius, 11<br />
Charcoal, 134<br />
Chelisoches morio, 215, 231<br />
Chemical activity, 236<br />
Chemical <strong>and</strong> biological controls,<br />
137<br />
Chemical arsenals, 189<br />
Chemical compounds, 76<br />
Chemical contaminants, 120<br />
Chemical control methods, 140<br />
Chemical control, 21, 34, 39, 41, 44,<br />
47, 49–51, 209, 269<br />
Chemical insecticides, 211, 217<br />
Chemical options, 313<br />
Chemical pesticides, 106, 283, 298<br />
Chemical treatments, 14, 74, 78, 79,<br />
86, 88, 93<br />
Chemicals, 39, 42, 49, 77, 216, 228<br />
Chemo-receptors, 224<br />
Cheyletus eruditus, 294<br />
Chilocorus kuwanae, 77<br />
Chilocorus bipustulatus, 38, 77, 79<br />
Chilocorus nigritus, 19, 77<br />
China, 43, 75, 83, 95, 168, 177, 178,<br />
284<br />
Chinese bitter orange, 3<br />
Chinotto, 4, 73<br />
Chios, 16, 18, 34, 37, 42, 44, 47, 55,<br />
57<br />
Chitin, 273, 291<br />
Chitinolytic enzymes, 273<br />
Chlorfenapyr, 44<br />
Chlorine, 294<br />
Chlorpyrifos, 21–25, 39, 47, 49, 50,<br />
67, 68, 77, 89, 97<br />
Chlorpyrifos-ethyl, 217<br />
Chlorpyrifos-methyl, 21–23, 25, 39,<br />
47<br />
Chorion, 80<br />
Choristoneura fumiferana, 241, 243,<br />
244, 245<br />
Choroedocus illustris, 193, 201, 202,<br />
203<br />
Chortoicetes terminifera, 179, 185<br />
Chromatomyia horticola, 84<br />
Chromosome, 316<br />
Chromotropic, 6<br />
Chronic bacterial infection, 259<br />
Chrysocharis pentheus, 86<br />
Chrysomphalus aonidum, 9, 74<br />
Chrysomphalus dictyospermi, 9, 19,<br />
23, 37, 62, 63<br />
Chrysomphalus pinnulifer, 10<br />
Chrysoperla carnea, 47<br />
Chrysopidae, 47<br />
Chytridiomycota, 260<br />
Chytrids, 260<br />
Cicadellidae, 7<br />
Cicindelidae, 70, 72<br />
Cidial, 217<br />
Cihexatin, 21<br />
Cilia, 286<br />
Ciliary arrangements, 286<br />
Ciliata, 286<br />
Ciliophora, 286<br />
Cirrospilus nr. lyncus, 86<br />
Cirrospilus diallus, 86<br />
Cirrospilus ingenuus (=Cirrospilus<br />
quadristriatus), 20<br />
Cirrospilus ingenuus, 20, 63<br />
Cirrospilus pictus, 43<br />
Cirrospilus quadristriatus, 43<br />
Cirrospilus vittatus, 86<br />
Cirrospilus, 43, 44<br />
Citron, 3, 29, 39, 47–50, 73<br />
Citrostichus phyllocnistoides, 20, 43,<br />
44, 63, 71, 81, 83–86, 98, 99<br />
Citrus aphids, 46, 67<br />
Citrus arthropod pest, 30
334<br />
INDEX<br />
Citrus aurantifolia, 3<br />
Citrus aurantium, 3, 29<br />
Citrus bergamia, 4, 29<br />
Citrus decumana, 4<br />
Citrus deliciosa, 3<br />
Citrus flower moth, 30<br />
Citrus flowers, 48<br />
Citrus gr<strong>and</strong>is, 3<br />
Citrus greening, 102, 103<br />
Citrus leafminer, 6, 29, 30, 42, 43,<br />
45, 58, 74, 80, 81, 85, 95, 96, 98<br />
Citrus limon, 3<br />
Citrus maxima, 3, 29<br />
Citrus mealybug, 6, 29, 36, 37, 38,<br />
39, 74, 87, 88<br />
Citrus medica, 3, 29<br />
Citrus myrtifolia, 4<br />
Citrus orchards, 61, 64–69, 72, 78,<br />
89, 101, 102, 107, 110, 114, 123,<br />
124<br />
Citrus paradisi, 3, 29<br />
Citrus pest management, 21, 27, 61<br />
Citrus pests, 15, 61–63, 69, 71<br />
Citrus red mite, 250, 252, 254, 267,<br />
273, 285, 297, 302, 307<br />
Citrus reticulata, 3, 29<br />
Citrus sinensis, 3, 29<br />
Citrus snow scale, 6<br />
Citrus Tristeza Virus, 74, 94<br />
Citrus whitefly, 29, 30<br />
Citrus, 3, 4, 6, 7, 12–14, 17, 21–23,<br />
25–51, 53–74, 76, 78–83, 85–99<br />
Cladosporium cladosporioides, 284,<br />
302<br />
Cladosporium, 284, 302<br />
Classical biological control programs,<br />
322<br />
Classical biological control, 15, 37,<br />
42, 61, 81, 106, 321<br />
Classification algorithms, 169<br />
Classification methods, 320<br />
Classification, 272<br />
Clay loam soils, 109<br />
Clays, 92, 95<br />
Clementine, 22, 73<br />
Cleonis punctiventris, 299<br />
Cleora fortunata, 10<br />
Clethodim, 144<br />
Climate, 74, 87, 312, 322<br />
Climatic conditions, 78, 81, 88, 93,<br />
311, 321<br />
Climatic events, 237<br />
Clofentezine, 21, 22, 24, 25, 53, 68<br />
Clover cover crops, 133<br />
Clover, 146, 147, 149, 151, 152<br />
Coccidae, 9, 17, 23, 29, 38, 55, 58<br />
Coccidea, 291<br />
Coccidia, 291, 306<br />
Coccidoxenoides perminutus<br />
(= Pauridia peregrina), 17<br />
Coccidoxenoides perminutus, 88<br />
Coccinella septempunctata, 46<br />
Coccinellid predator, 37, 38<br />
Coccinellid, 13, 14, 67<br />
Coccinellidae, 15–19, 38, 46, 47, 55,<br />
56, 61, 65, 77, 79, 87, 88, 134,<br />
153, 157, 160, 161<br />
Coccobius fulvus, 19<br />
Coccoidea, 36, 64, 68<br />
Coccophagus ceroplastae<br />
(= Aneristus ceroplastae), 17<br />
Coccus hesperidum, 9, 17, 23, 62<br />
Coccus pseudomagnoliarum, 9, 17,<br />
38, 74<br />
Coccus viridis, 9<br />
Coconut mite, 278, 279, 303, 308<br />
Coconut palm, 209<br />
Coconut trees, 279<br />
Coconut, 209, 210, 217, 232, 233<br />
Cocoon, 80, 211<br />
COII, 200, 205<br />
Coleoptera, 11, 61, 65, 70, 77, 79, 87,<br />
88, 92, 134, 157, 160, 161<br />
Collembola, 111<br />
Colloid surfaces, 114<br />
Colombia, 82<br />
Colomerus novahebridensis, 275<br />
Colonization, 237<br />
Colony health, 284, 305<br />
Colony, 75, 78, 87–89, 93, 237, 240,<br />
242, 243, 255, 284, 291, 292, 305<br />
Colorado Potato Beetle, 254
INDEX<br />
335<br />
Colour, 13<br />
Columbia University, 175, 176<br />
Commercial compounds, 23<br />
Commercial damage, 76<br />
Commercial production, 278, 293<br />
Commercially formulated EPNs, 107<br />
Commodities, 311<br />
Comperiella bifasciata, 19, 37, 63,<br />
77, 78, 98<br />
Computer simulations, 143<br />
Concentration, 217, 225, 226<br />
Confidor, 216<br />
Conidia, 141, 158, 261–263, 268,<br />
270–273, 277, 278, 284, 296, 305<br />
Conidial preparations, 278<br />
Conidiobolus brefeldionis, 264<br />
Conidiobolus coronatus, 262, 265<br />
Conidiobolus obscurus, 265<br />
Conidiobolus thromboides, 265<br />
Conidiobolus, 262, 264<br />
Conidiophore, 261–263, 272, 273,<br />
296<br />
Conidium, 262, 263, 296<br />
Conifer, 76<br />
Conjunctivitis, 236<br />
Conservation BC, 67, 70<br />
Conservation biocontrol strategies, 61<br />
Conservation biological control, 102,<br />
106<br />
Conservation, 62, 65, 70<br />
Constricting rings, 112, 115<br />
Consultants, 30, 42<br />
Control measures, 29, 30, 39, 47<br />
Control strategies, 312, 315, 320, 322<br />
Control tactic, 101, 103<br />
Control techniques, 5<br />
Control, 15–20, 29, 30, 32, 34–42,<br />
44, 45, 47–51, 53–57, 73, 74, 76,<br />
78, 79, 81, 86–89, 91–100, 133,<br />
134, 136–146, 149, 152–161, 249,<br />
251, 255, 269, 278–279, 281–285,<br />
292, 295, 296–299, 301–308<br />
Conveyor belt, 240<br />
Conyza canadensis, 143<br />
Cool season legumes, 137, 146, 147,<br />
149, 152<br />
Copper oxychloride, 217<br />
Copper sprays, 102<br />
Copper, 92, 95<br />
Cordyceps, 273<br />
Coreidae, 155<br />
Corfu, 15, 40, 58<br />
Cori<strong>and</strong>er, 92<br />
Corn, 254, 267, 279, 301, 301<br />
Cornuaspis beckii, 62, 63<br />
Corsica, 4, 15, 18, 19<br />
Cortical lesions, 76<br />
Corylus avellana, 283<br />
Cos, 42<br />
Cosmopterigidae, 84<br />
Cosmopterix pulchrimella, 84<br />
Cotesia robecula, 200, 201<br />
Cotton aphid, 75<br />
Cotton rolls, 33<br />
Cotton, 254, 267, 268, 270, 284,<br />
307<br />
Cottony egg masses, 13<br />
Cottony-cushion scale, 36, 38<br />
Cotyledons, 198, 203<br />
Cover crop management, 69<br />
Cover spaying, 34, 35<br />
Cowpea curculio, 154, 160<br />
Cowpea, 155, 199<br />
CPV, 216<br />
CPWC, 144<br />
Crabgrass, 143<br />
Crapemyrtle aphid, 153, 159<br />
Crataegus, 238<br />
Crawlers, 75, 79, 87, 99<br />
Crematogaster scutellaris, 11<br />
Crematogaster, 92<br />
Crete, 15–20, 30, 31, 32, 34, 37, 40,<br />
42, 43, 47, 49, 50, 54, 56, 57, 58<br />
Crimson clover, 146–152<br />
Cristulariella pyrimidalis, 141<br />
Criteria, 5, 21<br />
Critical period of weed control, 144<br />
CRM, 250, 251, 272, 273, 278, 285<br />
Crop cultivars, 107<br />
Crop protection practices, 70<br />
Crop, 13, 134–136, 141, 144, 146–150,<br />
152, 155–157, 158, 192, 193, 207,
336<br />
INDEX<br />
254, 255, 267–269, 292, 293, 297,<br />
298, 299, 305, 307<br />
Cropping systems, 312, 322<br />
Cropping, 113–115<br />
Crossvine, 76<br />
Crown gall, 141<br />
Crown, 210, 215, 241, 242<br />
Cryoprotective compounds, 268<br />
Cryptic habitats, 224<br />
Cryptoblabes gnidiella, 10<br />
Cryptochaetum iceryae, 63<br />
Cryptolaemus montrouzieri, 17, 25,<br />
37, 38, 63, 65, 67, 68, 88<br />
Crystal complex, 241<br />
Crystalline body, 254, 255<br />
Crystalline toxic body, 254<br />
Crystals, 252, 294, 301, 307<br />
CTV, 6<br />
Cultivar susceptibiltiy, 133<br />
Cultivars, 135, 137, 141–143, 154–156,<br />
158, 159<br />
Cultural control, 44<br />
Cultural practices, 4, 34, 36, 38, 40,<br />
41, 44, 48, 51, 108, 113, 114<br />
Cultural techiques, 39<br />
Culture media, 264, 270, 271, 283<br />
Curculio caryae, 138, 160<br />
Curculionidae, 11<br />
Cuticle, 112, 113, 129, 217, 263, 269,<br />
273, 278, 285, 286<br />
Cybocephalidae, 77<br />
Cybocephalus fodori, 38<br />
Cycle, 81, 82, 83, 84, 90<br />
Cyclopentanones, 200<br />
Cydia caryana, 138<br />
Cynodon dactylon, 143<br />
Cypermethrin, 21–26, 36, 39, 47, 49,<br />
138<br />
Cyperus, 143<br />
Cyprus, 43, 82, 83, 84<br />
Cystein protease, 196<br />
Cytopathological effects, 252<br />
Cytopathological studies, 253<br />
Cytoplasm, 251, 252, 253, 286<br />
Cytoplasmic incompatibility, 258,<br />
259, 303, 309<br />
Cytoplasmic polyhedrosis virus, 216<br />
Cytotoxic effects, 277<br />
Czech Republic, 268<br />
D<br />
Dactylellina dactyloides, 115<br />
Dactylellina haptotyla, 115, 126<br />
Dacus bait, 33<br />
Dagang, 178<br />
Damaeidae, 287–290<br />
Damaeus clavipes, 287, 288, 289<br />
Damaeus geniculatus, 287, 290<br />
Damaeus oblongus, 288, 290<br />
Damaeus onustus, 287, 288<br />
Damage categories, 178<br />
Damage, 48, 50, 239<br />
Damsel bugs, 148<br />
Danaus chrysippus, 260<br />
Darfur, 174<br />
Database, 67<br />
Datana integerrima, 134<br />
Date palm plantations, 220, 221<br />
Date palm, 210, 214, 215, 219–232<br />
Death, 253, 254, 261, 263, 277, 283,<br />
291<br />
Decomposition, 148, 149, 150<br />
Defense genes, 190, 191, 199, 200,<br />
204, 205<br />
Defense patterns, 202<br />
Defensive proteins, 199<br />
Defoliating Lepidoptera, 235<br />
Defoliation, 87, 134, 136, 155, 238<br />
Deformed wing virus, 254, 307<br />
Delphastus pusillus, 15<br />
Deltamethrin, 21–25, 92<br />
Demanyssidae, 286<br />
Demethylation inhibitors, 141<br />
Dendrocerus, 46<br />
Dendrolaelaps cornutus, 275<br />
Dendrolaelaps tetraspinosus, 275<br />
Dendrolaelaps, 265<br />
Density changes, 235, 316<br />
Density dependent pattern, 193<br />
Density, 5, 14, 220, 273, 283<br />
Dephosphorylation, 200<br />
Dermanyssoidea, 252, 308
INDEX<br />
337<br />
Dermanyssus gallinae, 257, 260, 302<br />
Dermaptera, 70, 215, 231<br />
Dermatitis, 236, 243, 244, 245<br />
Dermatophagoides pteronyssinus,<br />
256<br />
Desert locust habitats, 174, 175<br />
Desert locust, 164, 165, 170, 173–176,<br />
179, 182–187<br />
Desiccation, 284, 299<br />
Desmids, 261<br />
Detection, 13, 33, 36, 37, 39, 46, 53,<br />
249, 292, 293, 300<br />
Detergent, 14, 46<br />
Deterrent, 239<br />
Deuteromycetes, 260, 261, 272, 282,<br />
296, 307<br />
Deuteromycota, 272, 296, 298, 305<br />
Developing conservation biological,<br />
106<br />
Development, 6, 13, 76, 83, 84, 90,<br />
96, 312, 314, 315, 316, 317, 321,<br />
322, 324<br />
Developmental stages, 217<br />
Diachasma fullawayi, 20, 63<br />
Diachasmimorpha longicaudata, 20,<br />
63<br />
Diachasmimorpha tryoni, 20, 63<br />
Diaeretiella rapae, 46<br />
Diagnostic services, 119<br />
Dialectica scalariella, 84<br />
Dialeurodes citri, 8, 15, 23, 29–31,<br />
40, 54, 58, 74, 93, 99<br />
Dialeurodes citrifolii, 8<br />
Diameter, 14<br />
Diammonium phosphate, 92<br />
Diamond-back moth, 197<br />
Diapause, 177, 316<br />
Diaphorina citri, 74, 102<br />
Diaprepes abbreviatus, 101, 103–107,<br />
109, 110, 123–125, 127–130<br />
Diaprepes, 101, 103–105, 107, 109,<br />
110, 123–130<br />
Diarrhea, 250<br />
Diaspidid scales, 13<br />
Diaspididae, 9, 18, 23, 29, 30, 37, 62,<br />
63, 68, 75, 79, 96–99<br />
Diaspidids, 14<br />
Diaspidiotus perniciosus, 10<br />
Diazinon, 21, 22, 24, 25<br />
Diazinone, 217<br />
Dichlorvos, 21, 24<br />
Dicofol, 21, 22, 24, 25, 53, 68<br />
Dicrodiplosis, 87<br />
Dieback, 76<br />
Diflubenzuron, 21, 22, 24, 25, 139,<br />
161<br />
Digamasellidae, 265, 275<br />
Digital data, 167<br />
Digitaria, 143<br />
Diglyphus isaea, 86<br />
Dimethoate, 21–25<br />
Dinychus carinatus, 267<br />
Diospyros melanoxylon, 83, 95<br />
Diptera, 11, 29, 54–58, 62, 77, 84,<br />
87, 97<br />
Directive, 22, 26<br />
Dirhinus giffardii, 20, 33<br />
Discoloration, 294, 301<br />
Disease losses, 141<br />
Disease transmission, 321<br />
Disease, 5, 6, 102–104, 236, 244,<br />
249, 250, 251, 252, 253, 256, 258,<br />
259, 263, 264, 268, 271, 273, 281,<br />
283, 284, 291–295, 307, 308, 311<br />
Dispenser, 14<br />
Dispersal, 320, 321, 325<br />
Disruption, 12<br />
Distribution maps, 178<br />
Distribution, 108, 119, 124–127, 130,<br />
236, 237<br />
Dithiocarbamate, 5<br />
Ditylenchus dipsaci, 122<br />
Diurnal caterpillars, 191<br />
Diurnal insects, 192<br />
Diuron, 144<br />
Diversinervus elegans, 17, 37<br />
DMNT, 200<br />
DNA markers, 143<br />
DNA, 116, 118, 119, 120, 124, 125,<br />
127–130<br />
DNA-dependent RNA polymerase, 254<br />
Dociostaurus maroccanus, 181
338<br />
INDEX<br />
Dodine, 141, 142<br />
Dorsal ducts, 79<br />
Doses, 241<br />
Douglas Fir Tussock Moth, 239<br />
Downy Spot, 141, 142<br />
Dracaena, 76<br />
Droplets, 240<br />
Drosophila, 260<br />
Drought stressed plants, 194, 202<br />
Drought, 194, 202, 206, 261, 264,<br />
270<br />
Dryinidae, 15<br />
Dumbbell-shaped bodies, 294<br />
Dursban, 217<br />
Dusky stink bug, 155<br />
E<br />
Early detection, 163<br />
Earth surface, 164–167, 169<br />
Earth, 163, 185, 186<br />
Earwigs, 70, 215<br />
Ecesis, 83<br />
Echium, 84<br />
Ecological impact, 322<br />
Ecology, 101, 103, 123, 126<br />
Economic crop losses, 193<br />
Economic damage, 12, 281, 282<br />
Economic importance, 43, 93<br />
Economic injury level, 36, 38, 51<br />
Economic threshold, 5, 65, 66, 79,<br />
88, 250<br />
Ecosystem components, 189<br />
Ecosystem functioning, 189, 196<br />
Ecosystem processes, 190<br />
Ecosystem, 73, 86, 189, 193<br />
Ectomyelois ceratoniae, 10<br />
Ectoparasitic wasp, 84<br />
Ectoparasitoid, 77, 214<br />
Edaphic conditions, 106<br />
Egg predators, 239<br />
Egg sterilants, 104<br />
Egg, 75, 79–81, 83, 84, 87, 89–91,<br />
94, 104, 108, 109, 123, 209, 211,<br />
212, 214, 215, 229, 231, 239, 243,<br />
244, 252, 255, 258, 259, 292, 293<br />
Eggplant, 320, 325<br />
Egypt, 4, 27, 84, 96, 209, 210,<br />
215–217, 224, 231, 233<br />
Ehrlichieae, 257<br />
Elasmus flabellatus, 48<br />
Electromagnetic radiation, 165, 166,<br />
167<br />
Electromagnetic spectrum, 166, 167,<br />
172<br />
Eleusine indica, 143<br />
Elicitor defence genes, 200<br />
Elicitors, 189, 190, 191, 204<br />
Elutriation, 121<br />
Empoasca decedens, 7<br />
Empoasca, 7, 14<br />
Empresa Brasileira de Pesquisa<br />
Agropecuária, 271<br />
Encarsia (= Aspidiotiphagus)<br />
lounsburyi, 19<br />
Encarsia (= Prospaltella) perniciosi,<br />
19<br />
Encarsia (=Prospaltella) lahorensis,<br />
15<br />
Encarsia citrina, 38<br />
Encarsia herndoni (= Encarsia<br />
elongata), 19<br />
Encarsia herndoni, 19, 63<br />
Encarsia lahorensis, 15, 63<br />
Encarsia perniciosi, 19, 37, 63, 77<br />
Encarsia strenua, 63<br />
Encarsia, 260<br />
Encyrtid, 78, 81, 82, 88<br />
Encyrtidae, 18–20, 37, 38, 43, 48,<br />
65, 66, 71, 77, 81, 87, 88, 95, 99,<br />
100<br />
Endemic EPN species, 103, 108<br />
Endoparasitoids, 77, 78<br />
Endosymbionts, 259, 260<br />
Enterobacter, 256, 259<br />
Entomogenous fungi, 273<br />
Entomology, 133, 158<br />
Entomomophthorales, 261<br />
Entomopathogenic bacteria, 112<br />
Entomopathogenic nematodes, 101,<br />
103, 105, 110, 115, 123–129, 209<br />
Entomopathogens, 138<br />
Entomophagous arthropods, 50
INDEX<br />
339<br />
Entomophthora floridana, 267, 305,<br />
307, 309<br />
Entomophthora muscae, 262<br />
Entomophthoraceae, 261, 262, 301,<br />
304, 305, 309<br />
Entomophthoraceous infections, 267<br />
Entomophthoralean fungus, 263, 264,<br />
267<br />
Entomophthoralean species, 264<br />
Entomophthorales, 263, 297, 300–304,<br />
305<br />
Environment, 235, 236, 240, 241<br />
Environmental conditions, 35, 45,<br />
253<br />
Environmental hygiene, 236<br />
Environmental pollution, 269<br />
Enzymatic processes, 269<br />
Eotetranychus banksi, 266<br />
Eotetranychus hicoriae, 138<br />
Eotetranychus orientalis, 280<br />
Eotetranychus pueraricola, 260<br />
Eotetranychus sexmaculaturs, 265,<br />
276<br />
Eotetranychus suginamensis, 260<br />
Eotetranychus uncatus, 260<br />
Ephedrus persicae, 46<br />
Epidemics, 281, 282, 297, 298<br />
Epidemiological data, 222<br />
Epidermic reactions, 236<br />
Epistrophe baiteata, 46<br />
Epithelial cells, 251, 252, 293<br />
Epitremerus goniathrix, 273, 274,<br />
275<br />
Epizootic, 252, 269, 270, 271, 277,<br />
283, 302, 305, 306, 308<br />
EPN communities, 101, 103<br />
EPN distributions, 101, 107, 120<br />
EPN population, 101, 120<br />
EPN prevalence, 109, 113, 114, 116<br />
EPN spatial patterns, 114, 115<br />
EPN, 101, 103, 105–107, 109–116,<br />
123, 216, 224–230<br />
EPNs population biology, 101<br />
EPPO list, 6<br />
EPPO, 74, 98<br />
Equine encephalitis viruses, 252<br />
Eradication programs, 104<br />
Eretmocerus debachi, 16, 63<br />
Erhardovina bisphaera, 287<br />
Erhardovina carabodesi, 287<br />
Erhardovina euzeti, 287<br />
Erhardovina fuscozetesi, 287<br />
Erhardovina fuscozetis, 287<br />
Erhardovina oribatarum, 287<br />
Erhardovina phtiracari, 287<br />
Erhardovina platynothri, 287<br />
Erhardovina postneri, 287<br />
Erhardovina scutovertexi, 287<br />
Erhardovina, 287<br />
Eriophyes sheldoni, 11, 13, 299<br />
Eriophyidae, 11, 50, 54, 265, 273,<br />
281–283, 304, 305, 308<br />
Eriophyids, 249, 273, 278, 282, 297<br />
Eriophyiidae, 29, 30<br />
Eriophyiids, 50, 53<br />
Eriophyoidea, 274, 275, 308<br />
Eritrea, 173, 174<br />
Erosion, 149<br />
Erynia phalangicidae, 265<br />
Escharosis, 49<br />
Esfenvalerate, 138<br />
Establishment, 74, 82–86, 89, 92, 96,<br />
99<br />
Ethiopia, 173, 174<br />
Ethoprophos, 22<br />
Ethylene emission, 199<br />
Ethylene, 199, 200, 207<br />
Etiology, 252<br />
Etofenprox, 21, 22, 23, 24, 92<br />
Etoxazol, 21, 22, 24, 53, 68<br />
EU, 4, 62, 66, 67, 74, 241, 244<br />
Eucalymnatus tessellates, 9<br />
Eucalyptus blakelyi, 193, 206<br />
Eucalyptus, 238, 239<br />
Eucalyptus, 76<br />
Eucoilidae, 34, 57<br />
Eugregarine, 290<br />
Eugregarines, 290<br />
Eugregarinida, 289<br />
Eukaryotes, 286, 291<br />
Eukaryotic cells, 257<br />
Eulophid, 64, 83, 84, 85
340<br />
INDEX<br />
Eulophidae, 20, 38, 43, 44, 48, 55,<br />
58, 71, 81, 85, 97, 98, 99<br />
Eumaeus atala florida, 239<br />
Euonymus, 76<br />
Eupelopidae, 287<br />
Eupelops hirtus, 287<br />
Eupelops subuliger, 287<br />
Eupelops torulosus, 287<br />
Euphorbia species, 143<br />
Euphthiracaroidea, 289<br />
Eupodidae, 266<br />
Euproctis chrysorrea, 238<br />
Euproctis chrysorrhoea, 239, 241<br />
Euproctis edwardsii, 239<br />
Euproctis lunata, 239<br />
Euproctis pseuconspersa, 239<br />
Euproctis scintillans, 239<br />
Euproctis similis, 239<br />
Euproctis, 237, 239, 243, 245<br />
Eupterotidae, 236<br />
Europe, 237, 238, 240, 241, 292, 299<br />
European settlers, 135<br />
European silvopastoral systems, 135<br />
Euschistus servus, 155<br />
Euschistus tristigmus, 155<br />
Euseius addoensis, 319<br />
Euseius citrifolius, 265, 302<br />
Euseius elinae, 319<br />
Euseius finl<strong>and</strong>icus, 257, 260, 319<br />
Euseius fructicolus, 319<br />
Euseius sojaensis, 319<br />
Euseius stipulatus, 25, 51, 53, 54, 61,<br />
65–68, 71, 319<br />
Euseius tularensis, 319<br />
Euseius victoriensis, 319<br />
Eutetranychus banksi, 12, 24, 267,<br />
276, 309<br />
Eutetranychus orientalis, 12, 256,<br />
274, 276, 280<br />
Euzetes globulus, 287<br />
Euzetes seminulum, 287, 288, 290, 304<br />
Euzetidae, 287, 288<br />
EVA Green dye, 121<br />
Evaluation, 64, 66, 67<br />
Excretory <strong>org</strong>ans, 294<br />
Excretory products, 294<br />
Exochomus quadripustulatus, 38, 77,<br />
79<br />
Exotic arthropods, 74<br />
Exotic biological control, 61<br />
Exotic eulophids, 86<br />
Exotic IBCAs, 62, 70<br />
Exotic natural enemies, 81<br />
Exotic parasitoids, 33, 36<br />
Exotic pests, 74, 311<br />
Exotic species, 62, 74, 88<br />
Exotoxin, 254, 255, 303<br />
External morphology, 317<br />
Extraction, 121, 122<br />
Eyes, 89<br />
F<br />
Fagales, 133<br />
Fall armyworm, 199<br />
Fall webworm, 134<br />
Family, 256–258, 260, 262, 264, 269,<br />
274, 287, 301<br />
Far infrared, 166<br />
Farmed habitats, 106<br />
Farmers, 30, 33, 312, 314<br />
Farnesol, 22<br />
Fatbody, 253, 277<br />
Fatty acid potassium salt, 47, 50<br />
Fatty acid, 21–23<br />
Fecal pellets, 251<br />
Feces, 218, 227, 251, 255, 290<br />
Fecundity, 79<br />
Feeding sites, 79, 87<br />
Feeding specialization, 317<br />
Feeding, 77, 79–81, 83, 84, 86, 87,<br />
90, 93, 210, 212, 215, 224, 252,<br />
284, 286, 307, 317, 325<br />
Female mealybugs, 14<br />
Female, 75, 77, 79–83, 87, 90<br />
Feminization, 249, 258<br />
Fenazaquin, 21–25, 53, 68<br />
Fenbutatin oxide, 21, 22, 24, 25, 53,<br />
67, 68<br />
Fenitrothion, 21, 23–25<br />
Fenoxycarb, 21–25, 39, 44, 54<br />
Fenperoximate, 21–24, 53, 68<br />
Fermentation, 227
INDEX<br />
341<br />
Fern prothalli, 261<br />
Ferrugineol, 218, 232<br />
Ferrugineone, 218<br />
Fertilization process, 316<br />
Fertilization, 44, 73, 86, 87<br />
Fertilizer, 39, 45, 137, 146, 147, 149,<br />
153<br />
Festuca arundinacea, 69<br />
Ficus, 87<br />
Field experiments, 251, 279<br />
Field trials, 216, 218, 219, 223<br />
Fig wax scale, 75<br />
Filaments, 87<br />
Fire ant, 138, 154, 158–160<br />
Firmicutes, 260<br />
Fission, 263, 290<br />
Flagella, 260, 286, 291<br />
Flagellar action, 286<br />
Flagellata, 286<br />
Flagellates, 286<br />
Flatid planthoppers, 15<br />
Flatidae, 7, 15<br />
Flatwoods orchards, 109<br />
Flavedo, 285<br />
Flight, 13, 77<br />
Flooring, 134<br />
Florida citriculture, 102<br />
Florida citrus industry, 102<br />
Florida, 43, 54, 56, 81, 82, 84, 89,<br />
96–97, 101–104, 106, 107, 109,<br />
110, 112, 114, 115, 123–130, 250,<br />
267, 268, 273, 276, 300, 301, 302,<br />
305, 307–309<br />
Flower damage, 48<br />
Flower tissues, 48<br />
Flowering plants, 289<br />
Flowers, 13, 48, 49, 57<br />
Fluazifop, 144<br />
Fluctuation, 32, 40<br />
Flucythrinate, 22–25, 36, 39, 47, 49<br />
Flufenoxuron, 21, 22, 24, 25, 44, 45<br />
Flumioxazin, 144<br />
Fluorescence, 116<br />
Flushes, 13<br />
Flushing twigs, 13<br />
Fluted scales, 16<br />
Fluvalinate, 21, 22, 26<br />
Foliage, 39, 133, 136–139, 148, 155,<br />
161, 162, 241, 244<br />
Food attractant, 32, 32, 35<br />
Food availability, 311, 316<br />
Food, 6, 14, 62, 69, 250, 259, 261,<br />
286, 308<br />
Fopius arisanus, 63, 64<br />
Forecasting, 5<br />
Forest, 235, 236, 237, 238, 240, 244,<br />
245<br />
Forestry programs, 242<br />
Forestry, 236, 238, 245<br />
Forficulidae, 215, 231<br />
FormaSat, 168<br />
Formicidae, 11, 92, 95, 96<br />
Formothion, 217, 218<br />
Formulation, 134, 235, 240, 241, 243,<br />
244, 254, 283, 297, 299<br />
Fortuitous introduction, 74<br />
Fosalone, 25<br />
Fosetil-Al, 5<br />
Fowl pox virus, 252<br />
France, 4, 6, 7, 15–20, 27, 89, 93, 98,<br />
168, 176, 183–186, 209, 240, 241,<br />
244<br />
Frankliniella bispinosa, 7<br />
Frankliniella occidentalis, 7, 49,<br />
292<br />
Frass, 218, 227<br />
Fruit collection, 33<br />
Fruit flies, 20, 24<br />
Fruit juices, 102<br />
Fruit, 13, 29–36, 48–51, 54–58, 74,<br />
76, 79, 80, 87–92, 99, 133, 136,<br />
137, 143, 161<br />
Fruiting body, 260, 261<br />
Fuelwood, 134<br />
Fumagillin, 294<br />
Fumigants, 93<br />
Fumigation tablets, 217, 218<br />
Fungal diseases, 140<br />
Fungal pathogens, 249, 297, 298<br />
Fungi Imperfecti, 260, 296<br />
Fungi, 102, 111, 112, 114–116, 119,<br />
120, 125, 126, 129, 150, 161, 209,
342<br />
INDEX<br />
216, 249, 250, 260, 261, 264, 269,<br />
271–273, 282–285, 291, 296–298,<br />
299–306<br />
Fungicide, 5, 135–137, 141, 142,<br />
144, 156, 160<br />
Fungus, 216, 231, 261, 264, 267–271,<br />
277–284, 297, 299–300, 304–309,<br />
321<br />
Furniture, 134<br />
Fusarium, 296<br />
Fuscozetes setosus, 287<br />
Fusicladosporium effusum, 141<br />
G<br />
Galendromus annectes, 318<br />
Galendromus helveolus, 318<br />
Galendromus occidentalis, 63, 316,<br />
318<br />
Galeopsomyia fausta, 20, 63<br />
Galicia, 6<br />
Gametangia, 261<br />
Gametes, 260, 261, 290<br />
Gametogony, 290<br />
Gamma rays, 166<br />
Gamontocyst, 290<br />
Gamonts, 290, 291<br />
Gardenia, 87<br />
Gas, 218<br />
Gene, 254, 255, 296<br />
Genera, 272, 285, 296<br />
Generalist predators, 51<br />
Generalist, 317, 320, 323, 324<br />
Generations, 32, 42, 44, 45, 48, 50,<br />
51, 77, 79, 81, 87, 210<br />
Genus, 254, 258, 260, 262, 273, 292,<br />
296, 299–301, 304, 306, 309<br />
Geographic information system, 165,<br />
184<br />
Geometridae, 10<br />
Georeferenced data, 170<br />
Ge<strong>org</strong>ia, 4, 133, 136, 137, 141–145,<br />
152, 157–162<br />
Geospatial technologies, 163<br />
Germany, 240, 246<br />
Germination, 262, 263, 268, 270,<br />
284, 296, 297, 299, 306<br />
GIS, 163, 165, 169–171, 176,<br />
181–187<br />
Gl<strong>and</strong>s, 79, 236, 239<br />
Glass beads, 121<br />
Glass McPhail trap, 33<br />
Glasshouse, 255, 293, 312, 322<br />
Global Positioning Systems, 171<br />
Globodera artemisiae, 121<br />
Globodera pallida, 121<br />
Globodera rostochiensis, 121<br />
Globodera tabacum, 121<br />
Glomerella cingulata, 141<br />
Glucose-N-acetyl, 273<br />
Glue, 14<br />
Glufosinate, 144<br />
Glycerol, 268, 270, 279<br />
Glyphosate, 144, 145<br />
GMOs, 5<br />
Golgi apparatus, 285<br />
Goosegrass, 143, 283<br />
Government policies, 243<br />
GPS receiver, 171<br />
GPS, 165, 171, 176, 240<br />
Gracillariidae, 10, 20, 24, 60, 53, 54,<br />
57–58<br />
Grafted trees, 44<br />
Grafting, 135<br />
Granula, 295<br />
Granulosis viruses, 295<br />
Grape, 76<br />
Grapefruit flowers, 285<br />
Grapefruit, 3, 22, 29, 36, 39, 45, 47,<br />
49, 73, 76, 285<br />
Grass control, 133<br />
Grasshopper feeding, 172<br />
Grasshopper infestations, 171, 186<br />
Grasshopper, 171, 172, 177, 184–187,<br />
190, 193–195, 198, 202–204<br />
Gravid females, 65, 292<br />
Greece, 3–5, 7, 15–20, 21–23, 26–37,<br />
39–42, 44–51, 53–59, 82–84, 96, 97,<br />
209<br />
Green algae, 261<br />
Green lacewing, 46, 148<br />
Green leaf volatiles, 199, 200<br />
Green lemons, 251
INDEX<br />
343<br />
Green manures, 149<br />
Green stink bug, 154, 155, 159<br />
Green twigs, 13<br />
Greenhouses, 280, 281, 283, 292,<br />
297, 312<br />
Greening disease, 74<br />
Gregarina euzeti, 290<br />
Gregarina oribataram, 290<br />
Gregarina scutovertexi, 290<br />
Gregarina, 287, 289, 306<br />
Gregarines, 290, 291<br />
Gregarious behaviour, 237<br />
Ground cover mangement, 61, 69<br />
Ground cover, 61, 67, 69, 70<br />
Groundwater, 134, 149<br />
Groves, 85, 86, 92, 96, 99–104, 128,<br />
129, 135, 136, 155, 156<br />
Growers, 30, 35, 38, 40, 42, 67, 69,<br />
102, 133, 135–137, 139–143, 146,<br />
149, 152, 155<br />
Growing season, 13, 14, 140, 144<br />
Growth regulator insecticides, 139<br />
Guanine, 251, 294<br />
Guidelines, 4, 5, 6, 69<br />
Gulf of Aden, 173<br />
Gum, 76<br />
Gurleya sokolovii, 288<br />
Gut epithelium, 292<br />
Gymnoscelis pumilata, 10<br />
Gymnoscelis rufifasciata, 10<br />
H<br />
Habitat Mapping, 174, 177, 179<br />
Habitat, 163, 164, 171–175, 177,<br />
182–185, 194, 214, 222, 228, 230,<br />
237, 250, 319, 321<br />
Haemocoel, 216<br />
Hairs, 236, 237, 238, 239, 240, 243<br />
Halo, 263, 296<br />
Halosulfuron, 144<br />
Halotydeus destructor, 266<br />
Haploid cells, 260<br />
Haploid nuclei, 260<br />
Hardware, 164, 182<br />
Hardwoods, 134<br />
Harmful products, 67<br />
Harmonia axyridis, 16, 47, 55, 56,<br />
134, 138, 153, 161<br />
Harpoon, 236<br />
Harvest, 35, 36, 80, 92, 99<br />
Haustorium, 286<br />
Hazel, 283<br />
HBTM, 253<br />
Health hazards, 190<br />
Health-care, 236<br />
Helicopters, 240<br />
Helicoverpa armigera, 10<br />
Heliothis veriscence, 204<br />
Heliothrips haemorrhoidalis, 7, 29,<br />
49, 50, 58<br />
Hemiberlesia rapax, 10<br />
Hemiptera, 7, 29, 30, 37, 38, 40, 41,<br />
53, 55, 58, 62, 64, 66, 67, 75, 79,<br />
87, 95, 98, 99<br />
Hemipterans, 137, 139, 140, 155,<br />
156, 160<br />
Hemisarcoptes coccophagus, 274,<br />
280<br />
Hemisarcoptidae, 274, 280<br />
Hemocytes, 277<br />
Herbaceous plant, 68<br />
Herbicide runoff, 149<br />
Herbicides, 5, 137, 144–146<br />
Herbivores, 189–208, 272, 316, 320<br />
Herbivorous species, 191<br />
Herbivory, 189–191, 193–208<br />
Hermannia gibba, 287, 288<br />
Hermannioidea, 287, 288<br />
Heterodera glycines, 121<br />
Heterodera schactii, 121<br />
Heterorhabditidae, 224<br />
Heterorhabditids, 111, 112<br />
Heterorhabditis bacteriophora, 225,<br />
226, 229<br />
Heterorhabditis indica, 109, 112<br />
Heterorhabditis indicus, 225–227,<br />
229, 230<br />
Heterorhabditis zeal<strong>and</strong>ica, 109–112<br />
Heterorhabditis, 105, 110, 125, 127,<br />
216, 224, 225, 228, 230<br />
Heterotrophic <strong>org</strong>anisms, 150<br />
Hexythiazox, 21, 23, 24, 25, 67, 68
344<br />
INDEX<br />
Hibernation, 47<br />
Hickory shuckworm, 138<br />
Hickory, 134, 138–140, 143<br />
High plain virus, 252<br />
Hippodamia convergens, 194<br />
Hippodamia variegate, 46<br />
HIPV, 272<br />
Hirstionyssus, 286<br />
Hirsutella brownorum, 274<br />
Hirsutella danubiensis, 274<br />
Hirsutella gregis, 274<br />
Hirsutella haptospora, 274<br />
Hirsutella kirchneri, 274, 280, 281<br />
Hirsutella necatrix, 274, 281<br />
Hirsutella nodulosa, 275, 283<br />
Hirsutella rhossiliensis, 111<br />
Hirsutella rostrata, 275<br />
Hirsutella thompsonii, 273, 275–281,<br />
283, 299, 300<br />
Hirsutella tydeicola, 276<br />
Hirsutella v<strong>and</strong>ergeesti, 276<br />
Hirsutella, 273–274, 277, 278, 281,<br />
282, 296, 299–305, 308, 309<br />
Hirsutellin A, 277, 303, 304, 306<br />
Hirsutellin B, 277<br />
Historical data, 31<br />
Homoptera, 83, 96, 97, 98, 99, 262<br />
Homopteran pests, 64<br />
Homopteran, 64, 94<br />
Honduras, 82<br />
Honeybee tracheal mite, 253<br />
Honeybees, 80, 253<br />
Honeydew, 13, 46, 78, 87, 88, 93,<br />
134<br />
Horsenettle, 143<br />
Horseweed, 143<br />
Horticulture, 133<br />
Host spectrum, 251, 261, 264, 268,<br />
269, 283, 299<br />
Host, 105, 109, 127, 250, 251, 253,<br />
256, 258, 259, 260, 261, 262, 263,<br />
264, 268, 269, 270, 271, 273, 277,<br />
278, 283, 286, 287, 290, 291, 295,<br />
296, 299, 301, 302<br />
House fly, 215<br />
Hover flies, 148<br />
HtA, 277<br />
Huanglongbing, 6, 102<br />
Humeral bristles, 89<br />
Humidity, 81, 97, 263, 270, 283, 297,<br />
299, 306, 307<br />
Hungary, 89<br />
Hunting, 156<br />
Hurricanes, 164, 166<br />
Hydrachnellae, 287, 288, 303<br />
Hydrogen, 150<br />
Hydrolyzed protein, 33, 92<br />
Hylesia iola, 239<br />
Hylesia lineata, 239<br />
Hylesia urticans, 239<br />
Hylesia, 239, 244<br />
Hymenoptera, 11, 20, 27, 33, 34, 37,<br />
38, 40, 43, 44, 48, 54, 55, 57, 58,<br />
64–66, 71, 72, 77, 79, 81, 85, 87,<br />
88, 92, 94, 95–100<br />
Hyperparasitoids, 46<br />
Hyperspectral images, 167<br />
Hyphae, 260, 261, 263, 272, 273, 296<br />
Hyphal bodies, 261, 263, 264, 304<br />
Hyphantria cunea, 134<br />
Hyphomycetes, 272, 300, 305, 307<br />
Hypoaspis, 215<br />
Hypodermis, 277<br />
Hyponomeutidae, 10, 24, 30<br />
I<br />
IBCA (Invertebrate Biological<br />
Control Agents), 62<br />
Ice-nucleating substances, 268<br />
Icerya purchasi, 8, 13, 16, 36, 38, 62,<br />
63<br />
Icosahedral virus particles, 252<br />
Iflavirus, 254, 306<br />
Imagery, 170, 172, 174–176, 183,<br />
186, 187<br />
Imidacloprid, 21–25, 45, 67, 77<br />
Immature stages, 211, 215<br />
Immigration, 83, 85<br />
Immune system, 253<br />
Importation, 74, 92<br />
Inclusion bodies, 250, 255, 295<br />
Incompatibilities, 249, 296, 300
INDEX<br />
345<br />
Incubation period, 215<br />
Incubation, 215<br />
India, 83, 93, 168, 173, 174, 185,<br />
189, 209, 215, 216, 232, 233, 267,<br />
278, 299, 305, 307, 308<br />
Indigenous food webs, 62<br />
Indigenous parasitoids, 38, 86<br />
Indigenous predators, 322<br />
Indochinese peninsula, 75<br />
Indonesia, 83, 209, 210, 232<br />
Industrial production, 278<br />
Industrial repellent, 154<br />
Infection periods, 142<br />
Infection routes, 250<br />
Infection, 91, 104, 105, 111, 129,<br />
250, 251, 252, 259, 267, 268, 269,<br />
270, 271, 273, 278, 282, 283,<br />
290–291, 293, 302, 303, 306<br />
Infectious propagule, 263<br />
Infective juvenile, 105, 113<br />
Infective stage, 290, 291<br />
Infestation, 30, 32, 35, 38–44, 46, 48,<br />
49, 51, 53, 55, 57, 75, 76, 78, 79,<br />
81, 85–89, 91, 92, 99, 209, 210,<br />
215–217, 220, 222, 223, 226, 227,<br />
229, 232, 235<br />
Infrared photos, 167<br />
Inhalation, 236<br />
Injection, 217, 226, 227, 233, 277,<br />
284<br />
Inoculation, 65<br />
Inoculum, 141, 152, 157<br />
Insect attack, 189, 193, 201, 203,<br />
204, 207<br />
Insect cadaver, 111, 112, 250<br />
Insect death, 106<br />
Insect grazing, 194<br />
Insect growth regulators, 77, 86<br />
Insect pest, 6, 14–20, 53, 134, 139,<br />
146, 148, 153, 209<br />
Insect, 6, 14–20, 53, 64, 69, 71, 133,<br />
134, 136–138, 142, 146–148,<br />
153–156, 160–162, 189–199, 201,<br />
203–205, 206, 207, 211, 249, 250,<br />
254, 260, 261, 277, 283, 295, 297,<br />
299, 300, 303, 305, 307, 323, 324<br />
Insectary, 78<br />
Insecticidal soap, 138<br />
Insecticidal sprays, 222<br />
Insecticide, 5, 21, 23, 27, 33, 35, 36,<br />
39, 41, 42, 44, 45, 47–50, 78, 86–87,<br />
89, 96, 101, 102, 104–105, 133,<br />
136–139, 142, 154, 209, 211, 216,<br />
217, 227, 230, 231, 232, 285<br />
Insect-plant interactions, 194<br />
Inspections, 3, 6, 13, 46<br />
Instar larvae, 82, 215, 221<br />
Instar, 75, 76, 78, 80, 82, 83, 84, 85,<br />
90–91, 215, 224, 225<br />
Insulaspis gloverii, 62, 63<br />
Integrated control programs, 249,<br />
285, 299<br />
Integrated control strategies, 74, 77<br />
Integrated Pest Management, 4, 29,<br />
42, 101, 102, 296, 312 (see also:<br />
IPM)<br />
Integrated production, 4<br />
Integument, 250, 284, 286<br />
International Institute for Tropical<br />
Agriculture, 271<br />
International Pheromone Plastic<br />
McPhail trap, 32<br />
Internet, 183, 184<br />
Intestine, 106, 224<br />
Intexta acarivora, 288, 292, 304<br />
Intracellular bacteria, 296<br />
Intracellular gram-negative bacteria,<br />
257<br />
Intracellular symbionts, 249, 260<br />
Intraguild predation, 321<br />
Intrauterine, 216<br />
Introduced eulophids, 86<br />
Introduced parasitoids, 106<br />
Introduction, 29, 73–74, 78, 81, 92,<br />
94, 311, 313, 314, 321–322<br />
Inundative releases, 297<br />
Invasion, 40, 41<br />
Invertebrate biological control agents,<br />
61, 62, 70<br />
Invertebrate pathology, 249, 254<br />
Invertebrate pests, 296–297<br />
IP, 4–6, 26
346<br />
INDEX<br />
Iphiseius (Amblyseius) degenerans,<br />
50<br />
Iphiseius degenerans, 50, 51, 319<br />
IPM strategy, 53<br />
IPM, 3, 4, 5, 6, 29, 36, 39, 41, 45, 47,<br />
49, 51, 53, 57, 63, 66–69, 71, 72,<br />
101–102, 103, 104, 121–123, 209,<br />
230, 232, 233, 249, 311–314<br />
IPMT, 32, 33, 36<br />
Ipomoea, 143<br />
Iran, 173<br />
Irrigation, 39, 44, 45, 73, 86, 87, 137,<br />
145, 153, 159<br />
Irritation, 239<br />
IRS 1C, 168<br />
IRS 1D, 168<br />
IRS ResourceSat, 168<br />
Isaria fumosorosea, 299<br />
Ismailia governorate, 211<br />
Israel, 4, 5, 81–84, 94, 209, 232,<br />
243<br />
Istamine, 239<br />
<strong>Italy</strong>, 3–5, 7–12, 15–20, 23, 24, 27,<br />
50, 71, 73–74, 80–85, 87, 91–94,<br />
209, 235, 238, 240, 241, 242, 243,<br />
283<br />
Itching, 239<br />
ITS region, 118<br />
ITS1, 129<br />
ITS2, 129<br />
J<br />
JA (jasmonic acid), 197, 198, 199,<br />
200, 201, 202, 204<br />
Japan, 83, 168, 239, 260, 267, 305<br />
Japanese bayberry whitefly, 40, 94,<br />
98<br />
Jasmine, 87<br />
Jasmonate, 198, 200, 202, 203, 205<br />
Jasmonic acid, 197<br />
Jojoba, 79<br />
Jordan, 209, 232<br />
Jugl<strong>and</strong>aceae, 133<br />
Juice processing, 102<br />
Jujube, 76<br />
Juvenile, 113, 253, 255, 269<br />
K<br />
Kairomone, 219, 222, 230<br />
Kampimodromus aberrans, 319, 323,<br />
325<br />
Kaolin, 21, 92<br />
Kazakhstan, 177, 178, 181, 182, 185,<br />
187<br />
KBV (Bee Kashmir Virus), 253, 307<br />
Kelly's citrus thrips, 49, 50<br />
Kernel spot, 155<br />
Kernel-feeding hemipterans, 155<br />
Kerosene, 217<br />
Kingdom Fungi, 260<br />
Kiwi, 79<br />
Korinthia, 43, 58<br />
Kuwait, 209, 231<br />
L<br />
Label, 68<br />
Laboratory colonies, 252, 258, 259,<br />
294<br />
Laboratory production, 278<br />
Laboratory protocols, 119–120<br />
Laboulbeniales, 286<br />
La<strong>by</strong>rinthomorpha, 289<br />
Lacewing, 77, 81<br />
Laconia-Peloponnese, 42<br />
Ladder rungs, 134<br />
Ladybeetle, 77, 148, 153<br />
Lakonia, 43<br />
Lambda-cyhalothrin, 21–25, 92<br />
L<strong>and</strong>sat 168, 172<br />
L<strong>and</strong>sat ETM+ data, 178, 187<br />
L<strong>and</strong>sat Thematic Mapper data, 174,<br />
185<br />
L<strong>and</strong>scape, 134, 151, 240<br />
Larix decidua, 237<br />
Larva, 80, 81, 84, 85, 89, 211, 224,<br />
225, 226<br />
Larvae, 80–84, 90–92, 104, 105,<br />
108, 109, 111, 125, 128, 129, 208,<br />
210, 211, 214–218, 224–227, 229,<br />
236–243<br />
Larval feeding, 198<br />
Lasiocampidae, 236, 244<br />
Lasius alienus, 89
INDEX<br />
347<br />
Lasius niger, 11<br />
Latin America, 252, 269, 271<br />
Leaf cuticle, 81, 85<br />
Leaf miner, 64, 68<br />
Leaf proteins, 193<br />
Leaf skeletonizer, 238, 244<br />
Leaf wetness, 141, 156<br />
Leaf yellowing, 76<br />
Leaf-axils, 226, 228, 229<br />
Leaffooted bugs, 155<br />
Leafhoppers, 14<br />
Leafminer development, 81<br />
Leafroller, 75<br />
Leaves, 40, 43, 46, 51, 79, 81, 93,<br />
241, 243<br />
Lecanicillium lecanii, 298, 299<br />
Legs, 87, 89<br />
Legumes, 137, 146–152, 161<br />
Leguminous plants, 147<br />
Lemon, 12, 22, 26–27, 32, 36, 39, 45,<br />
47–50, 73, 74, 75, 76, 82, 91, 95,<br />
96, 98<br />
Lemons, 48, 49, 51, 61, 251<br />
Leonidion, 47<br />
Lepidoptera, 10, 30, 53–55, 58, 80, 83,<br />
84, 87, 95–99, 134, 196, 235–239,<br />
243–245, 254, 260<br />
Lepidopteran defoliators, 240, 241<br />
Lepidopteran infestations, 240<br />
Lepidopteran pests, 139<br />
Lepidopterism, 239, 245<br />
Lepidopterous pests, 133, 254<br />
Lepidosaphes beckii, 10, 19, 23, 30,<br />
31, 36, 37<br />
Lepidosaphes gloverii, 10, 19<br />
Leptinotarsa decemlineata, 254<br />
Leptoglossus oppositus, 155<br />
Leptoglossus phyllopus, 155<br />
Leptomastidea abnormis, 38, 87, 88<br />
Leptomastix dactylopii, 16, 25, 37,<br />
50, 59, 63, 65, 71, 88, 97, 99, 100<br />
Lestodiplosis aonidiellae, 77<br />
Lesvos, 42, 44<br />
Leucopis, 87<br />
Liacaroidea, 288<br />
LIDAR, 167<br />
Life cycle, 209, 211, 216, 241, 290,<br />
291<br />
Life style, 311, 313, 317–320<br />
Liguria, 15<br />
Lima bean, 199–202, 205, 206<br />
Limacodidae, 236<br />
Limantriidae, 239<br />
Lime, 3<br />
Limnochares aquatica, 287, 288, 290,<br />
303<br />
Linepithema (=Iridomyrmex) humile,<br />
11<br />
Linoleic acid, 199<br />
Linolenic acid, 199, 205<br />
Lipid, 200<br />
Liriomyza, 84<br />
Lobes, 79<br />
Locomotion, 214, 286<br />
Locust breeding areas, 163, 174, 175,<br />
177, 179, 187<br />
Locust egg-pods, 169<br />
Locust habitat monitoring, 163, 174,<br />
183, 184–186<br />
Locust habitat, 170, 172, 174, 175,<br />
179, 182, 185<br />
Locust nymphal development, 164<br />
Locust outbreaks, 163, 164, 172, 175<br />
Locust plagues, 164, 172, 179, 186,<br />
187<br />
Locust swarm, 164, 175<br />
Locusta migratoria burmana, 177<br />
Locusta migratoria capito, 177<br />
Locusta migratoria cinerescens, 177<br />
Locusta migratoria manilensis, 173,<br />
174<br />
Locusta migratoria migratoria, 177<br />
Locusta migratoria migratorioides,<br />
177<br />
Locusta migratoria, 177, 187<br />
Locusts, 163, 165, 170, 172, 174–177,<br />
179, 181–188<br />
Longevity, 211<br />
Lopholeucaspis japonica, 10<br />
Loquat, 76, 90<br />
Lorryia formosa, 276<br />
Lotus corniculatus, 196, 205
348<br />
INDEX<br />
Louisiana, 82<br />
Lufenuron, 21–25<br />
Lumber, 134<br />
Lycenidae, 239<br />
Lycosidae, 70<br />
Lymantria dispar, 240–241, 244<br />
Lymantriidae, 236, 243, 244<br />
Lyophilization, 121<br />
Lysiphlebus confusus, 46<br />
Lysiphlebus fabarum, 46<br />
Lysiphlebus testaceipes, 16, 25, 46,<br />
63, 65, 67, 68<br />
Lysis buffer, 120<br />
Lysis, 120, 253<br />
Lyxus algirus, 11<br />
M<br />
Macrocheles, 260, 264, 305<br />
Macrochelidae, 264<br />
Macrosiphum euphorbiae, 8, 45<br />
Macrosiphum mentzeliae, 194<br />
Madagascar, 181, 185<br />
Madeira Isl<strong>and</strong>, 6, 12, 74<br />
Magnesium sulphate, 119<br />
Magnolia, 76<br />
Maize, 193, 196, 199, 200, 201, 202,<br />
208<br />
Malacosoma californicum pluviale,<br />
194<br />
Malaria, 286, 290<br />
Malathion, 21–25<br />
Male killing, 249, 258<br />
Males, 218, 221–224, 228, 229<br />
Mali, 174, 187<br />
Malpighian tubes, 294<br />
Malpighian tubules, 277, 294<br />
Malta, 6<br />
Mammals, 135, 189<br />
Managed habitats, 106<br />
Management practices, 38, 44, 47<br />
Management regimes, 114<br />
Management, 101, 102, 103, 106,<br />
113, 123, 124, 128, 163, 164,<br />
170–172, 176, 178, 181–182, 183,<br />
184, 185, 187, 197, 199, 205,<br />
311–314, 320, 322, 323<br />
M<strong>and</strong>arin, 3, 22, 29, 35, 36, 39, 42–43,<br />
47, 49, 71, 76<br />
M<strong>and</strong>uca sexta, 197, 204<br />
Mango, 76<br />
Maple tree, 76<br />
Marathon, 47<br />
Margarodidae, 8, 38<br />
Maritime Alps, 241<br />
Mass production, 264, 297, 298<br />
Mass rearing, 314<br />
Mass trapping, 211, 223<br />
Mastigophora, 286<br />
Mating disruption, 138<br />
Mato Grosso, 281<br />
Mature female, 75<br />
Maturity, 35, 79, 91, 94<br />
Mauritania, 174, 183, 185–187<br />
Mealybug, 14, 24, 29, 30, 36, 37, 87,<br />
88, 96<br />
Mechanical damage, 197, 199, 200,<br />
207<br />
Mechanical harvester, 135<br />
Mechanical processes, 269<br />
Mechanical wounding, 197<br />
Medfly, 6, 31–36, 59, 64, 68<br />
Mediterranean areas, 91<br />
Mediterranean basin, 6, 62, 64, 67,<br />
74, 79, 81, 87, 89, 92, 94, 97<br />
Mediterranean black scale, 30, 36<br />
Mediterranean climates, 241<br />
Mediterranean countries, 45, 64, 66,<br />
91, 96<br />
Mediterranean fruit fly, 29–31, 54,<br />
56–58, 62, 64, 72, 89, 90, 91<br />
Mediterranean region, 3, 4<br />
Mediterranean, 3, 4, 6, 7, 26<br />
Medlure, 92<br />
Megalopygidae, 236<br />
Meiosis, 260, 286, 290<br />
Meira argovae, 285<br />
Meira geulakonigii, 285, 301<br />
Melanocallis caryaefoliae, 134, 159<br />
Melanocallis caryaefoliella, 138<br />
Meliaceae, 194<br />
Meloidogyne fallax, 130<br />
Meloidogyne incognita, 129
INDEX<br />
349<br />
Meloidogyne javanica, 120, 124<br />
Melon aphid, 75<br />
Member states, 21, 241<br />
Membranes, 257, 262, 277 286<br />
Mentzelia punila, 194<br />
Merculiaris annua, 84<br />
Merozoites, 290<br />
Metabolism, 195<br />
Metalaxyl, 5<br />
Metaphycus bartletti, 37<br />
Metaphycus helvolus, 37, 63<br />
Metaphycus lounsburyi<br />
(= Metaphycus bartletti), 18<br />
Metaphycus lounsburyi, 18, 63<br />
Metaphycus swirskii, 18, 37<br />
Metarhizium anisopliae, 283, 299,<br />
304<br />
Metarhizium, 283, 296, 301, 304<br />
Metaseiulus arboreus, 318<br />
Metaseiulus citri, 318<br />
Metaseiulus occidentalis, 252, 254–257,<br />
289, 292, 299, 304<br />
Metaseiulus pomi, 318<br />
Metazoa, 286<br />
Metcalfa pruinosa, 7, 15<br />
Meteorological data, 30<br />
Meteorological models, 175<br />
Meteorological parameters, 172<br />
Meteosat, 172<br />
Methomyl, 21–25, 33, 44<br />
Methoxyfenozide, 21, 22, 24, 45<br />
Methyl anthranilate, 154<br />
Methyl carbitol, 154<br />
Methyl jasmonate, 202–203<br />
Methyl myristate, 154<br />
Methylcyclohexanecarboxylic acid,<br />
92<br />
Metronidazole, 294<br />
Mexico, 82, 89, 133, 135, 143, 159,<br />
181, 182, 278, 279<br />
Microbial miticide, 255<br />
Microbial products, 241<br />
Microbiological identification, 257–258<br />
Micrococcaceae, 255–256<br />
Microcosm assays, 112<br />
Microlysis, 121<br />
Micro<strong>org</strong>anisms, 92, 227, 249, 250,<br />
257, 258, 322<br />
Microscopic surveys, 258<br />
Microsphaera penicillata, 141<br />
Microspora, 288, 289, 290, 291, 299,<br />
301, 304, 308<br />
Microsporidia, 249, 291–294<br />
Microsporidiosis, 291, 293, 300<br />
Microsporidium phytoseiuli, 288,<br />
301<br />
Microsporidium, 288, 291, 292, 300,<br />
304<br />
Microterys nietneri, 63<br />
Microtritia minima, 289<br />
Microwave, 166<br />
Mid infrared, 166<br />
Middle East, 74, 89, 181<br />
Midgut, 251, 252, 277, 290, 291<br />
Migratory locust, 177, 178, 179,<br />
182<br />
Millet, 155<br />
Mine, 80, 81<br />
Mineral oil, 21–25, 67, 68, 79, 89<br />
Mint, 92<br />
Minute pirate bug, 148<br />
Miridae, 7<br />
Mirrors, 236<br />
Mississippi, 268, 307<br />
Mite pest, 50, 249, 250, 280, 281<br />
Mite predators, 133, 156<br />
Mite, 13, 24, 29, 30, 50, 51, 53, 54, 56,<br />
57, 66, 68, 75, 102, 111, 126, 133,<br />
136–140, 151, 152, 154, 156–158,<br />
192, 199–202, 249–260, 264–267,<br />
269–272, 274–275, 277–285, 287,<br />
289–300, 311, 313, 316, 318–321,<br />
322, 323, 324, 325<br />
Miticide, 136, 137, 139<br />
Mitochondria, 285, 291<br />
Mitosis, 254<br />
Mitosomes, 291<br />
Model, 31, 142, 143, 161<br />
MODIS data, 178<br />
MODIS, 168, 172, 175, 176, 178,<br />
185–188<br />
Moericke pan-traps, 14, 46
350<br />
INDEX<br />
Moisture, 146–148, 150, 151<br />
Mole cricket, 106<br />
Molecular beacon, 121<br />
Molecular detection, 119<br />
Molecular methods, 111, 285<br />
Molecular techniques, 120, 249, 291,<br />
293, 295<br />
Mollicutes, 260<br />
Monellia caryella, 134, 138, 158,<br />
159, 161<br />
Monelliopsis pecanis, 134, 138, 159,<br />
161<br />
Monieza expansa, 290<br />
Moniliaceae, 284<br />
MONITOR-E-1, 168<br />
Monitoring, 6, 13, 14, 30, 32–37, 39,<br />
43, 45–49, 51, 55, 77, 78, 79, 96,<br />
139, 155–157, 163, 167, 169, 172,<br />
174, 175, 178, 180–183, 236, 240,<br />
312, 313, 321<br />
Monoclonal antibodies, 293<br />
Mononychellus tanajoa, 262, 265,<br />
266, 268, 276, 302, 305, 306<br />
Mononychellus, 262, 265, 266, 274,<br />
276, 300, 302, 305<br />
Montenegro, 4, 7<br />
Moraceae, 194<br />
Morningglories, 143<br />
Morocco, 4, 26, 82, 83, 84, 98<br />
Morphology, 236, 240<br />
Mortality, 139, 140, 142, 160, 216,<br />
217, 224–228, 240, 254, 255, 267,<br />
271, 277, 279, 281, 283, 284, 285,<br />
298, 306, 307, 317<br />
Mosquitoes, 290<br />
Moth, 20, 30, 196, 197, 206, 237,<br />
238, 239, 240, 241, 243, 244<br />
Moult, 236<br />
Moulting, 75<br />
Mouth parts, 250<br />
Mouth, 211, 212<br />
Mucosal tissues, 236<br />
Mucous substance, 261, 263<br />
Mucous tissues, 236<br />
Mud, 216<br />
Mulberry, 76, 79<br />
Multicolored asian ladybeetle, 134,<br />
139, 153<br />
Multiplex systems, 120<br />
Mummies, 270<br />
Mummified cadaver, 272<br />
Mummy, 264<br />
Musca domestica, 215<br />
Muscle tissue, 253, 292<br />
Muscles, 277<br />
Mutualism, 259<br />
Mutualistic bacteria, 224<br />
Mycelial preparations, 278<br />
Mycelium, 261, 263, 272, 278, 286<br />
Mycetaspis personata, 10<br />
Mycorrhizae, 150<br />
Mycosed aphids, 283–284<br />
Mycosphaerella caryigena, 141<br />
Mycotoxins, 261<br />
Myrtle-leaved orange, 4<br />
Myxospora, 289<br />
Myzus ornatus, 8<br />
Myzus persicae, 8, 45, 53, 55<br />
N<br />
Napamichum aequifolium, 288<br />
Native st<strong>and</strong>s, 134, 135, 136<br />
Natural enemies, 5, 6, 12, 26, 37–42,<br />
44–48, 51, 53, 55, 57, 61, 63, 64, 66,<br />
67, 68, 69, 70, 72, 74, 77, 78, 81, 87,<br />
88, 93, 94, 97, 102, 104, 110, 111,<br />
115, 123, 128, 137, 153, 154, 156,<br />
158, 209, 212, 214, 313, 321<br />
Natural mortality, 281<br />
Natural <strong>org</strong>anisms, 5<br />
Natural resources, 164<br />
Near infrared, 166<br />
Neem extract, 154<br />
Nelson Isl<strong>and</strong>, 268<br />
Nematode infection, 224, 225, 229<br />
Nematode suspension, 226–228<br />
Nematodes, 101, 105, 109, 110, 112,<br />
113, 115, 116, 119, 120, 123–130,<br />
209, 216, 224–233<br />
Nematophagous fungi, 111<br />
Neochrysocharis formosa, 43, 44,<br />
86
INDEX<br />
351<br />
Neodryinus typhlocybae, 15<br />
Neogregarines, 290<br />
Neogregarinida, 289<br />
Neomyzus circunflexum, 8<br />
Neonicitinoid insecticides, 138<br />
Neoseiulus barkeri, 257, 319<br />
Neoseiulus bibens, 257, 318<br />
Neoseiulus californicus, 65, 66, 70,<br />
315, 316, 318, 320–325<br />
Neoseiulus cucumeris, 252, 288, 292,<br />
316, 319<br />
Neoseiulus fallacis, 318<br />
Neoseiulus idaeus, 318<br />
Neoseiulus longispinosus, 318, 320<br />
Neoseiulus tiki, 318<br />
Neoseiulus umbraticus, 319<br />
Neoseiulus, 252, 257, 260, 271, 276,<br />
288, 292, 305<br />
Neozygitaceae, 261–263, 302, 304<br />
Neozygites abacaridis, 265, 305<br />
Neozygites acaricida, 266<br />
Neozygites acaridis, 266, 305<br />
Neozygites adjarica, 267, 302<br />
Neozygites cf. acaridis, 268<br />
Neozygites floridana, 264, 266–269,<br />
297, 301–302, 304, 305, 308, 309<br />
Neozygites tanajoae, 262, 266, 268–271,<br />
298, 302, 303<br />
Neozygites tetranychi, 266<br />
Neozygites tetranychid, 266<br />
Neozygites, 262–269, 272, 297, 298,<br />
301–306<br />
Nephus (Sidis) anomus, 17<br />
Nephus bisignatus, 38, 56<br />
Nephus includens, 38, 56<br />
Nephus quadrimaculatus, 17<br />
Nephus reunioni, 37, 88<br />
Nephus sidi, 37<br />
Nepticulidae, 83, 84<br />
Nerium ole<strong>and</strong>er, 67<br />
Nerolidol, 22<br />
Nest, 237, 241<br />
Nesting sites, 134, 151<br />
New South Wales, 179, 184<br />
Newly formed fruits, 48<br />
Nezara viridula, 7, 155<br />
Nicotiana sylvestris, 197, 207<br />
Nicotiana tabacum, 191<br />
Nifedipine, 294<br />
Nipaecoccus nipae, 9<br />
Nitidulid, 38<br />
Nitrogen fertilizer, 52<br />
Nitrogen partitioning, 203<br />
Nitrogen, 52, 133, 136, 137, 146–149,<br />
152, 153, 160, 161<br />
NOAA-GOESS, 168<br />
Noctuidae, 10, 236<br />
Nolidae, 238, 244<br />
Nomadacris septemfasciata, 181<br />
Nomuraea rileyi, 299<br />
Nonselective acaricide, 254<br />
Nonsexual spores, 261<br />
Norflurazon, 144<br />
Normalized Difference Vegetation<br />
Index, 173<br />
North America, 238, 240<br />
North Carolina, 267, 283, 299<br />
Nosema acari, 288<br />
Nosema euzeti, 288<br />
Nosema führeri, 288<br />
Nosema helminthorum, 288<br />
Nosema hermanniae, 288<br />
Nosema ptyctimae, 288<br />
Nosema sperchoni, 288<br />
Nosema steganacari, 288<br />
Nosema steinhausi, 289<br />
Nothroidea, 287, 288, 289<br />
Nothrus silvestris, 288, 306<br />
Notodontidae, 134, 239, 245<br />
Notostrix attenuata, 274<br />
Notostrix formosae, 275<br />
Nozzle, 240<br />
Nuclei, 251, 252, 253, 261, 286, 292,<br />
295<br />
Nucleotide sequence, 260<br />
Nucleus, 251, 277, 285<br />
Nursery, 12, 22, 24, 43–45, 47, 61,<br />
65, 66, 74, 86<br />
Nut crop, 134, 135, 136<br />
Nut production, 133, 135, 136<br />
Nutsedge, 143<br />
Nymph, 41, 140, 215
352<br />
INDEX<br />
Nymphal distribution, 164<br />
Nymphal exuviae, 75, 79<br />
Nymphal habitats, 178<br />
Nymphalidae, 11, 236<br />
O<br />
Oak Processionary Moth, 237, 245<br />
Oak st<strong>and</strong>s, 237<br />
Oak, 76, 237, 238, 240, 244<br />
Ocellar bristles, 89<br />
Ochrogaster lunifer, 239, 244<br />
Octadecanoid pathway, 191, 201<br />
Octadecanoid signal pathway, 191<br />
Oenopia (Synharmonia) conglobata,<br />
41, 46<br />
Oenothera laciniata, 144<br />
Offshoots, 210, 215, 216<br />
Offspring, 259, 291, 296, 316<br />
Ohio, 114, 115<br />
Oil palm, 209, 218, 223, 231, 232,<br />
233<br />
Oklahoma, 142, 148, 159, 161<br />
Ole<strong>and</strong>er scale, 74, 79<br />
Ole<strong>and</strong>er, 76, 79, 87<br />
Olfactory cues, 90<br />
Oligonychus biharensis, 256<br />
Oligonychus gossypii, 266, 271, 276,<br />
281<br />
Oligonychus hondoensis, 266, 267, 305<br />
Oligonychus ilicis, 276<br />
Oligonychus pratensis, 266, 302<br />
Oligosporidium occidentalis, 289,<br />
293<br />
Olive black scale, 75<br />
Olive, 76, 79<br />
Oman, 82, 83, 84<br />
Onion, 196<br />
Ontogeny, 296<br />
Oocysts, 290<br />
Oomycetes, 104<br />
Oozing, 217<br />
Opius concolor, 33<br />
OPM, 237, 240, 241, 242, 243<br />
Oral secretion, 189–191, 199, 204<br />
Orange spiny whitefly, 74<br />
Orange trees, 33, 42<br />
Orange, 3, 22, 29, 32–36, 39, 42–43,<br />
47, 49, 61<br />
Orbiliales, 119, 129<br />
Orchard fauna, 74<br />
Orchard, 6, 14, 22, 26, 27, 31, 33–43,<br />
45–47, 49–51, 54, 55, 58, 65, 67,<br />
68, 70, 72, 74, 77, 78, 82, 85, 86,<br />
88, 89, 92–97, 99, 102, 103, 105,<br />
107, 109, 110, 112, 115, 124, 125,<br />
127, 133–137, 140–158, 161, 179,<br />
252, 268<br />
Orchid fleck virus, 252<br />
Orchid, 252<br />
Organelles, 285, 290<br />
Organic matter, 114, 133, 137, 147,<br />
149, 150<br />
Organochlorine soil pesticides, 105<br />
Organochlorine, 5<br />
Organophosphate insecticides, 138, 139<br />
Organophosphates, 89, 96<br />
Organs, 13<br />
Oribatid mite, 290, 306<br />
Oriental migratory locust, 178<br />
Ornamental plants, 76<br />
Ornamentals, 104<br />
Orthezia insignis, 8<br />
Ortheziidae, 8<br />
Orthoptera, 7<br />
Oryctes rhinoceros, 212, 232<br />
Oryzalin, 144<br />
Oshin, 216<br />
Osmotic pressure, 262<br />
Otiorrhynchus aurifer, 11<br />
Outbreak, 29, 36–39, 41, 45, 47, 50–51,<br />
136, 139, 153, 156, 163, 164,<br />
171–173, 178, 179, 181, 182, 184,<br />
186, 188, 235, 236, 237, 238, 242,<br />
278<br />
Outdoor crops, 297<br />
Ovarial development, 269<br />
Ovary, 291, 293<br />
Overgraftings, 43, 48<br />
Overwintering, 32, 58<br />
Oviposition, 90–92, 195, 196, 204,<br />
211, 212, 252, 254, 269, 277,<br />
294
INDEX<br />
353<br />
Ovipositor, 89<br />
Ovisac, 87<br />
Oxalis pes-caprae, 68<br />
Oxamyl, 23, 24, 47, 50<br />
Oxydemeton-methyl, 21, 23, 24, 25<br />
Oxythyrea funesta, 11<br />
P<br />
Pachyneuron aphidis, 46<br />
Pachyneuron vindemmiae, 92<br />
Pachyneuron, 46<br />
Paecilomyces eriophytis, 282<br />
Paecilomyces farinosus, 283<br />
Paecilomyces lilacinus, 283<br />
Paecilomyces, 282, 283, 296<br />
Paenibacillus nematophilus, 112<br />
Paenibacillus, 112, 113, 116, 125<br />
Pakistan, 83, 173, 174<br />
Palaearctic region, 237<br />
Palestine, 209<br />
Palm stems, 218<br />
Palm tissues, 211, 218, 219, 222<br />
Palm tree, 209–211, 218–220, 222,<br />
224, 226–229, 231, 232<br />
Palm, 76, 79, 209–212, 216–219,<br />
222, 226, 229, 230, 232, 233<br />
Panonychus ulmi, 53, 250, 251<br />
Panonychus citri, 12, 13, 24, 29, 30,<br />
50, 51, 54, 56, 61, 62, 65, 66, 68,<br />
74, 250, 254, 265, 266, 267, 274,<br />
276, 280, 307<br />
Pantomorus cervinus, 11<br />
Paper envelope, 33<br />
Paper folded traps, 33<br />
Parabemisia myricae, 8, 40, 41, 56,<br />
74, 93, 94, 98<br />
Paraffin oil, 39, 41, 45, 47, 49, 53<br />
Paragus albifrons, 46<br />
Paraleyrodes bondari, 8<br />
Paraleyrodes citricolus, 8<br />
Paraleyrodes minei, 8<br />
Parapheromone, 32, 33, 92<br />
Paraquat, 144<br />
Parasaissetia nigra, 9<br />
Parasitic females, 216<br />
Parasitic fungi, 260<br />
Parasitic wasps, 191, 201, 207<br />
Parasitidae, 264, 265, 266, 267<br />
Parasitiformes, 274<br />
Parasitism levels, 34<br />
Parasitism, 13<br />
Parasitization, 84–86, 92–95, 99<br />
Parasitoid species, 37, 38, 42, 43<br />
Parasitoid, 7, 14, 26, 27, 33, 34, 36–46,<br />
48, 54–58, 64, 65, 67, 71, 78, 81–89,<br />
92, 93, 94–99, 209, 214, 224, 239,<br />
243<br />
Paratheresia menezesi, 214<br />
Paratrichodorus pachydermus, 122<br />
Pardosa cribata, 70, 72<br />
Parietaria diffusa, 84<br />
Parlatoria perg<strong>and</strong>ii, 62, 75, 94<br />
Parlatoria ziziphi, 10, 23<br />
Paros, 42<br />
Parthenogenesis, 94, 249, 258, 309<br />
Parthenogenetic biotypes, 79<br />
Parthenogenetic development, 261<br />
Parthenolecanium persicae, 9<br />
Particles, 250–253, 304, 307<br />
Paspalum notatum, 143<br />
Paste, 217, 218<br />
Pathogen, 250, 251, 258, 267, 268,<br />
271, 272, 278, 290–293, 295–297,<br />
301–306, 307<br />
Pathogenesis, 259<br />
Pathogenic fungi, 250, 268, 302<br />
Pathogenicity, 142, 225, 227, 230,<br />
255, 283, 283, 284, 297, 306<br />
Pathogens, 197, 200, 202, 205, 206,<br />
215, 249, 250, 261, 262, 271, 272,<br />
285, 287, 291, 292, 295, 296,<br />
299–301, 303, 305–307, 309<br />
PCR buffer, 120<br />
PCR template, 120<br />
PCR, 120<br />
Peach, 76, 79, 90, 91, 252, 306<br />
Pear, 31, 75, 76, 79, 90<br />
Pecan aphids, 134, 136, 139, 140,<br />
148, 152, 157, 159, 162<br />
Pecan leaf scorch mite, 136, 138,<br />
139, 158<br />
Pecan nut casebearer, 138–140
354<br />
INDEX<br />
Pecan trees, 134, 136, 144, 146, 148,<br />
154, 155, 160<br />
Pecan weevil survival, 139<br />
Pecan weevil, 136, 138–140, 152,<br />
154, 156<br />
Pecan, 133–149, 151–162<br />
Peloponnese, 20, 30, 36, 42, 43, 47,<br />
48, 49<br />
Pendimethalin, 144<br />
Penetration, 236, 250, 263, 269, 273,<br />
277<br />
Pentatomidae, 7, 138, 155<br />
Penthaleidae, 266<br />
Penthaleus major, 266<br />
Pepper, 320, 325<br />
Pergamasus crassipes, 264<br />
Pergamasus, 264–267<br />
Peridroma saucia, 10<br />
Persimmon, 87, 90<br />
Perturbance, 314<br />
Peru, 82<br />
Pest control, 5, 6, 236, 243, 311, 313<br />
Pest infestations, 311<br />
Pest management practices, 102, 123<br />
Pest management, 137, 148, 152,<br />
156, 157, 158, 160<br />
Pest outbreaks, 136, 140<br />
Pest species, 250, 283<br />
Pest, 3, 5, 6, 7, 13, 21, 25–32, 36–42,<br />
44–46, 48, 49, 51, 53, 55, 56–58,<br />
59, 61, 62, 63, 64, 65, 67, 68, 71,<br />
72, 74, 76, 77, 79, 86–88, 90, 91,<br />
93, 94–96, 98, 101–107, 110,<br />
123–125, 127, 133, 136–140, 148,<br />
153, 154, 156, 158, 160, 189, 192,<br />
193, 200, 201, 203, 204, 206, 250,<br />
255, 268, 269, 280, 281, 292, 296,<br />
297, 308, 309<br />
Pesticide applications, 4<br />
Pesticide groups, 5<br />
Pesticide list, 39<br />
Pesticide treatments, 102<br />
Pesticide, 3, 5, 6, 21, 25, 26, 32, 36,<br />
61, 66, 67, 71, 101, 102, 104, 106,<br />
128, 133, 135–137, 155, 156, 190,<br />
192, 203, 204, 207, 312, 322<br />
Petrobia hartii, 68<br />
Petroleum oil, 39, 47, 49, 53, 102<br />
Pezothrips kellyanus, 49, 50<br />
Pezothrips kellyanus, 7, 29, 49, 50,<br />
54, 58, 74<br />
Phaenacoccus madeirensis, 9<br />
Phaenoglyphis, 46<br />
Phaneroptera nana, 7<br />
Phaseolus lunatus, 199, 206<br />
Phasmarhabdites hermaphrodita,<br />
122<br />
Pheidole pallidula, 89<br />
Phenological changes, 182<br />
Phenthoate, 217<br />
Pheromone dispensers, 77<br />
Pheromone trap, 77, 79, 88, 214,<br />
218–222, 229, 231<br />
Pheromone, 14, 77, 78, 81, 91, 96<br />
Phialid, 277<br />
Phialides, 273<br />
Phialidic conidiogenesis, 296<br />
Phialidic conidiogenous cell, 296<br />
Phloem sap, 93<br />
Phoenix canariensis, 211<br />
Phomalactone, 277<br />
Phosalone, 22<br />
Phosmet, 21–25, 36, 39, 92, 138<br />
Phosphonate potassium, 5<br />
Phosphorous, 150, 294<br />
Phosphorylation, 200<br />
Photoperiod, 316<br />
Photorhabdus, 105, 224<br />
Phthiracaroidea, 287–289<br />
Phthiracarus globosus, 287, 288<br />
Phthiracarus piger, 287, 289<br />
Phthiracarus, 287, 288, 289<br />
Phyla, 260, 289<br />
Phyllocnistis citrella, 6, 10, 24, 29–31,<br />
42, 53–54, 56–58, 62–64, 71, 72,<br />
74, 80–86, 94–99<br />
Phyllocoptruta oleivora, 11, 24,<br />
273–275, 277, 280, 299, 301, 306<br />
Phylogenetic studies, 291<br />
Physiological <strong>and</strong> behavioural<br />
responses, 319<br />
Physiological changes, 191
INDEX<br />
355<br />
Physiological mechanisms, 316<br />
Physiological processes, 254<br />
Physotritia duplicata, 289<br />
Phytohormone, 197<br />
Phytonemus pallidus, 275<br />
Phytophagous mites, 139, 315<br />
Phytophagous populations, 240<br />
Phytophthora cactorum, 141<br />
Phytophthora nicotianae, 104<br />
Phytophthora palmivora, 104<br />
Phytophthora, 103, 105, 107, 124,<br />
125<br />
Phytoprotection, 200, 206<br />
Phytopthora Shuck <strong>and</strong> Kernel Rot,<br />
141<br />
Phytoptus avellanae, 283<br />
Phytoregulators, 73<br />
Phytosanitary control, 78<br />
Phytoseiid mites, 5, 68<br />
Phytoseiid releases, 321<br />
Phytoseiid, 50, 53, 251, 292, 293,<br />
294, 304, 314, 316, 317, 320, 321,<br />
322, 323, 324, 325<br />
Phytoseiidae, 50, 54, 56, 61, 66, 69,<br />
71, 77, 256, 257, 264, 265, 269,<br />
276, 280, 288, 289, 292, 299–302,<br />
307, 308<br />
Phytoseiulus longipes, 318<br />
Phytoseiulus macropilis, 318<br />
Phytoseiulus persimilis, 65, 66, 70,<br />
252, 254–257, 265, 288, 292–294,<br />
299, 300, 301, 306–308, 315, 316,<br />
318, 320, 322, 323, 325<br />
Phytoseius macropilis, 319<br />
Phytoseius spoofi, 319<br />
Picorna-like viruses, 253<br />
Pieris brassicae, 191<br />
Pieris rapae, 196, 200<br />
Pigeon Pea Mosaic virus, 252<br />
Pigweed, 143<br />
Pimetrozine, 23<br />
Pine Processionary Moth, 237<br />
Pine, 202, 237<br />
Pinus canariensis, 237<br />
Pinus halepensis, 237<br />
Pinus laricio, 237<br />
Pinus nigra austriaca, 237<br />
Pinus pinaster, 237<br />
Pinus pinea, 237<br />
Pinus sylvestris, 237<br />
Piridaben, 21, 23, 25, 68<br />
Pirimicarb, 21–23, 25, 47, 67, 68<br />
Pirimiphos-methyl, 21–23, 68<br />
Pistacia lentiscus, 83<br />
Pittosporum, 87<br />
Planococcus citri, 6, 9, 14, 24, 29–31,<br />
36, 51, 56, 62, 63, 65, 66, 71, 74,<br />
87–89, 96, 99<br />
Plant biomass, 189, 193, 204<br />
Plant breeders, 135<br />
Plant composition, 32<br />
Plant defense genes, 200<br />
Plant defense, 191, 193, 194, 205,<br />
207<br />
Plant elicitor, 197<br />
Plant growth regulators, 5<br />
Plant invasion, 311<br />
Plant pathogens, 285<br />
Plant pathology, 133<br />
Plant protection products, 5, 21, 26,<br />
36, 39, 41, 45, 47, 49, 50, 53<br />
Plant Protection Services, 30, 31, 35,<br />
36<br />
Plant protection, 5, 21, 26, 30, 31, 54<br />
Plant tissue, 250<br />
Plant volatiles, 190, 191, 195, 204,<br />
205, 207, 255<br />
Plantation, 219–222, 230<br />
Planting, 5<br />
Plant-inhabiting mites, 250, 280<br />
Plasmodium vivax, 286<br />
Plastic buckets, 218<br />
Plastic McPhail trap, 32<br />
Platygastridae, 16<br />
Platynothrus peltifer, 287, 289<br />
Pleistophora cephei, 289<br />
Pleistophora dindali, 289<br />
Pleistophora oribatei, 289<br />
Pleistophora platynothri, 289<br />
Pleistophoridae, 292, 300<br />
Plugs, 258, 259, 294<br />
Plywood, 134
356<br />
INDEX<br />
Pnigalio agraules, 85<br />
Pnigalio pectinicornis, 43, 44, 55<br />
Pnigalio soemius, 44, 58, 86<br />
Poaceae, 69<br />
Poales, 69<br />
Pol<strong>and</strong>, 267, 300, 305<br />
Polar filament, 291, 293<br />
Polar tube, 291<br />
Pollen, 236<br />
Pollution, 5<br />
Polyhedra, 295<br />
Polypeptide, 255, 277<br />
Polyphagotarsonemus latus, 12, 275,<br />
280, 283, 305, 306<br />
Pomelo, 22<br />
Poor condition, 294<br />
Population biology, 110, 123<br />
Population density, 14, 32, 51, 235,<br />
250, 251, 273, 283, 306, 314<br />
Population dynamics, 316, 321<br />
Population equilibrium, 205<br />
Population fluctuation, 222<br />
Population levels, 32, 34, 39, 46, 47<br />
Population size, 32, 250<br />
Population, 74, 77, 79, 86, 88, 92, 94,<br />
98<br />
Populations balance, 314<br />
Porosity, 109, 110, 113, 114<br />
Portugal, 4–7, 11, 15–20, 26, 74, 83,<br />
85, 96<br />
Potassium salts, 21, 23<br />
Potassium, 21, 22, 23, 294<br />
Potato-dextrose agar, 284<br />
Pothos, 87<br />
Poultry red mite, 260, 302<br />
Powdery mildew, 141<br />
PPM, 237, 241<br />
Praecocilenchus ferruginophorus, 216<br />
Praon volucre, 46<br />
Pratylenchs neglectus, 121<br />
Pratylenchs penetrans, 121<br />
Pratylenchs thornei, 121<br />
Pratylenchus zeae, 120, 124<br />
Prays citri, 10, 14, 24, 30, 31, 37, 38,<br />
48, 49<br />
Predaceous mites, 311, 313, 324<br />
Predaceous stink bugs, 148<br />
Predation, 110, 112, 115, 116, 119,<br />
123<br />
Predator, 7, 13–14, 37–39, 41, 45–47,<br />
51, 53, 56, 57, 65, 67, 77, 79, 87,<br />
88, 92, 95, 189–192, 194, 196,<br />
200–204, 207, 209, 215, 224, 231,<br />
249, 252, 254, 255, 259, 271, 290,<br />
292–294, 299, 303, 306, 307, 311,<br />
313–317, 319–321, 323, 324<br />
Predator-predator interactions, 323<br />
Predatory beetles, 77, 79<br />
Predatory insect, 189, 190<br />
Predatory mite, 53, 249, 250, 252,<br />
254, 255, 258, 260, 269, 271, 281,<br />
285, 292, 293, 298, 299, 300, 303,<br />
306, 307<br />
Prenuptial association, 290<br />
Prepollination, 141, 142<br />
Prepupae, 84<br />
Pre-pupal stage, 211<br />
Prevalence, 271, 281, 294, 304<br />
Prey densities, 317, 318<br />
Prey, 38, 47, 252, 255, 259, 290,<br />
292–293, 304, 315, 319<br />
Prey-predator system, 321<br />
Primary conidia, 261<br />
Primary conidium, 263<br />
Primary leaf, 203<br />
Primary productivity, 203<br />
Primer targets, 118<br />
Primers, 116, 118, 120, 124, 129<br />
Privet, 76<br />
Probe, 118<br />
Probes, 116, 118, 124, 129<br />
Procida, 16, 17<br />
Proctolaelaps, 275<br />
Prodinychidae, 267<br />
Product amplification, 116<br />
Production, 45, 48, 50, 61, 66, 133,<br />
135–137, 139, 140, 142, 143,<br />
147–149, 153, 156–158, 160, 162<br />
Progeny, 259, 294<br />
Proline, 193, 194, 202<br />
Pronematus, 274<br />
Propagation, 270
INDEX<br />
357<br />
Propargite, 21, 22, 24, 25, 68<br />
Propilus syagris, 274<br />
Propylea quatuordecimpunctata, 46<br />
Protease inhibitor, 199<br />
Protected crops, 69<br />
Protein hydrolysate, 32, 33, 35<br />
Proteinaceous bodies, 250<br />
Proteinase K, 120<br />
Proteobacteria, 137<br />
Protista, 286<br />
Protocols, 5<br />
Protoplasm, 262, 292<br />
Protopulvinaria pyriformis, 9<br />
Protozoa, 286, 287, 290, 306<br />
Pruning, 39, 44, 45, 73, 79, 89, 141<br />
Pseudo-arrhenotoky, 317<br />
Pseudococcidae, 9, 24, 29, 56, 66, 71<br />
Pseudococcus calceolariae, 9, 74<br />
Pseudococcus longispinus, 9<br />
Pseudococcus viburni, 9<br />
Pseudomonas aeruginosa, 215, 231<br />
Pseudomonas putida, 255, 256, 300<br />
Pseudomonas syringae, 197, 205<br />
Pseudopodia, 286<br />
Psyllidae, 83<br />
Psylliodes chrysocephala, 198<br />
Psyttalia concolor, 92<br />
Psyttalia incisi (= Opius incisi), 21<br />
Psyttalia incisi, 21, 63<br />
Pteromalidae, 38, 81, 92<br />
Public hygiene, 236<br />
Pulp, 90<br />
Pulvinaria floccifera, 9<br />
Pumelo, 3, 29, 39, 49<br />
Pupa, 80, 85, 90, 211, 214, 225<br />
Pupae, 90, 214, 215, 217, 225<br />
Pupal cell, 80<br />
Pupal stage, 81, 82, 91<br />
Pupation, 237<br />
Putrescine, 32<br />
Pygidium, 79<br />
Pymetrozine, 21–23, 47, 68<br />
Pymotidae, 215<br />
Pyralidae, 10<br />
Pyrethrines, 22, 23, 47<br />
Pyrethroid insecticides, 5<br />
Pyrethroid, 92<br />
Pyridaben, 22, 24, 53<br />
Pyrimiphos-methyl, 23–25<br />
Pyriproxifen, 21–23, 25, 68, 77<br />
Pyroglyphidae, 256<br />
Q<br />
qPCR, 116–120, 124, 127<br />
Quadrastichus citrella, 20, 63, 81, 82<br />
Quadrastichus, 20, 43, 44<br />
Quail, 151, 156<br />
Qualitative damage, 49<br />
Quantitative PCR, 116<br />
Quarantine pests, 6<br />
Quarantine, 6, 26, 41, 42, 45, 62, 64,<br />
74, 84, 92, 97, 104, 138<br />
Queensl<strong>and</strong>, 179, 184<br />
Quercus cerris, 238<br />
QUIAmp DNA mini kit, 121<br />
R<br />
RADAR, 167, 180, 182<br />
Radiation, 165, 166, 167<br />
Radiometric resolution, 167<br />
Rainfall, 140, 141, 142, 149, 151,<br />
159, 164, 169, 173–176, 268, 281,<br />
283<br />
RAMSES, 176<br />
Rapeseed, 197<br />
Raphanus raphanistrum, 196<br />
Rating, 317<br />
Ratzeburgiola incompleta, 86<br />
rDNA, 118, 268, 296<br />
Real time qPCR, 118<br />
Real-time PCR, 116, 126, 128<br />
Rearing, 64, 209, 211, 292, 293,<br />
314–315<br />
Recovery, 217, 226, 227<br />
Rectum, 258, 294<br />
Red alders, 195<br />
Red Palm Weevil, 209, 230–232<br />
Red ring disease, 223, 231–233<br />
Red Sea, 173, 176<br />
Red spider mite, 74<br />
Reflectance, 165, 166<br />
Registration, 21, 139, 224
358<br />
INDEX<br />
Regression model, 271<br />
Regulation, 249, 250<br />
Regulatory measures, 42<br />
Relative humidity, 65, 263, 270, 271,<br />
277, 283, 296, 297, 299<br />
Release, 15–20, 62, 64–66, 214, 215,<br />
217, 221, 230<br />
Remote sensing satellites, 163, 167, 183<br />
Remote sensing technology, 164<br />
Remote sensing, 163, 164, 165, 167,<br />
169, 172, 174, 175, 177, 179, 181,<br />
182–188<br />
Renibacterium salmoninarum, 256<br />
Repellents, 154<br />
Replication, 291<br />
Reproduction, 39, 44, 50, 79, 98, 192,<br />
258, 260, 261, 272, 286, 290, 292,<br />
301, 317<br />
Reproductive potential, 250<br />
Reproductive tissue, 258<br />
Research programs, 314<br />
Reservoir plants, 67<br />
Residual toxicity, 67<br />
Resistance genes, 143<br />
Resistance, 6, 137, 141, 143, 156–158,<br />
190, 192, 196–198, 200, 206, 207<br />
Resolution, 167, 168, 172, 174–176,<br />
178, 181, 182, 186<br />
Resting spores, 261, 262, 264, 270,<br />
296, 298<br />
Resurgence, 138, 139, 156, 157<br />
Retracus elaeis, 275, 308<br />
Retracus johnstoni, 274, 284<br />
Reversed plastic cups, 33<br />
Revision, 22<br />
Rhizobia, 151<br />
Rhizobiaceae, 137<br />
Rhizobial inoculant, 151<br />
Rhizobiales, 137<br />
Rhizoglyphus robini, 280<br />
Rhizoids, 263, 264<br />
Rhizopoda, 286<br />
Rhodes, 42<br />
Rhododendron, 87<br />
Rhodolia cardinalis, 38, 63, 67, 68<br />
Rhopalosiphum maidis, 8, 45<br />
Rhopalosiphum padi, 69<br />
Rhynacus, 275<br />
Rhynchophorus vulneratus, 218, 223<br />
Rhynchophorus ferrugineus, 209, 210,<br />
212, 214–216, 218–220, 222–225,<br />
228, 229–232<br />
Rhysotritia ardua, 287, 288, 306<br />
Rhyzobius (= Lindorus) lophanthae,<br />
19<br />
Rhyzobius forestieri, 17, 37, 55<br />
Rhyzobius lophanthae, 38, 63, 77,<br />
79<br />
Ribosomal DNA, 118, 130<br />
Ribosomal RNA gene, 289<br />
Ribosome-inhibiting proteins, 277<br />
Rickettsia, 259<br />
Rickettsiaceae, 257, 258<br />
Rickettsiales, 258, 309<br />
Rickettsia-like infections, 258<br />
Rickettsia-like <strong>org</strong>anisms, 257–259<br />
Rickettsieae, 257<br />
Rickettsiella phytoseiuli, 256, 308<br />
Rind bleaching, 50<br />
Ripening, 32, 35<br />
Risk assessment, 30, 163, 175, 182<br />
Risk rating, 138, 154, 159<br />
Rivers, 165, 177<br />
RNA synthesis, 254<br />
Roads, 165, 170<br />
Robinia pseudoacacia, 239, 244<br />
Rodolia (= Novius) cardinalis, 16<br />
Rodolia cardinalis, 25, 38, 61, 63<br />
Romalea guttata, 196<br />
Root weevil, 101, 104, 106, 107, 109,<br />
110, 124, 125, 127, 129<br />
Root-knot nematodes, 112<br />
Roots, 104, 105a, 127<br />
Rosaceae, 238<br />
Rostrum, 211, 212<br />
Rotenone, 22–24<br />
Royal palm, 209<br />
RPW larvae, 215, 225<br />
RPW, 209–212, 214–230<br />
Rubber plantations, 281, 282<br />
Rubber tree leaves, 281<br />
Rubber tree, 281
INDEX<br />
359<br />
Rubus ulmifolius, 83, 84<br />
Rural community, 135<br />
Ryegrass, 152<br />
S<br />
Sac, 260, 261<br />
Sago palm, 209<br />
Sahel, 173<br />
Saissetia coffeae, 9<br />
Saissetia oleae, 9, 18, 23, 29, 30, 31,<br />
36–39, 55, 62, 63, 75, 94<br />
Salicylic acid, 200<br />
Saliva, 76<br />
Salix alba, 83<br />
Salvinia molesta, 198, 206<br />
Samea multiplicalis, 198, 206<br />
Samos, 42<br />
Sample, 109, 110, 115, 117, 119–121,<br />
124, 126, 127<br />
Sampling methods, 119<br />
Sampling schemes, 37<br />
Sampling, 6, 26, 30, 31, 33, 37, 40,<br />
43, 46–49, 51, 53, 55<br />
S<strong>and</strong>, 107–109, 112, 114, 115<br />
Sap exudated, 210<br />
Sap, 73, 76, 210, 217, 222, 226<br />
Saprophytes, 115<br />
Sapsucking insects, 89<br />
Sarcomastigophora, 289<br />
Sardinia, 15, 16–18<br />
Satellite images, 164, 172, 174<br />
Satellite-derived information, 178<br />
Satellites, 164, 165, 167, 168, 171,<br />
172, 174, 176, 178, 182, 183<br />
Saturation point, 263, 297<br />
Saturniidae, 236, 239<br />
Saudi Arabia, 74, 89, 173, 186, 209,<br />
210, 215, 216, 225, 228, 230–233<br />
Scab control, 141<br />
Scab epidemics, 142<br />
Scab resistance, 143<br />
Scaeva albomaculata, 46<br />
Scale insects, 30, 36–39<br />
Scale population, 77<br />
Scale, 29, 30, 36–39, 42, 62, 75–79,<br />
94–99<br />
Scanners, 166<br />
Scapteriscus, 106<br />
Scarabaeidae, 11<br />
Scarring, 49, 50<br />
Schistocerca piceifrons piceifrons, 181<br />
Schistocerca, 170, 173, 183, 185,<br />
186, 188<br />
Schizogony, 290<br />
Scolia erratica, 214<br />
Scutellista cyanea, 38<br />
Scutellum, 89<br />
Scutovertex minutus, 287, 290<br />
Scutoverticidae, 287<br />
Scymnus, 79, 87<br />
Scymus (Pullus) subvillosus, 46<br />
Season, 268, 270, 271, 278, 282, 297,<br />
298<br />
Secondary conidia, 261, 262, 296<br />
Secondary conidium, 263<br />
Secondary hosts, 257<br />
Secondary infestations, 91<br />
Secondary metabolic products, 191<br />
Secondary metabolism, 200, 205<br />
Seed formation, 147<br />
Seedling trees, 135<br />
Seedlings, 136<br />
Segments, 211<br />
Seiulus, 276<br />
Selective insecticides, 44, 48<br />
Semielacher petiolatus, 18, 43, 44,<br />
81, 83–86, 97, 98<br />
Semielacher silvicola, 44, 58<br />
Semiochemicals, 89<br />
Senescence, 294<br />
Sensor, 167, 172, 175<br />
Sentinel weevils, 111<br />
Septa, 260, 261, 296<br />
Sequences, 268, 296<br />
Serangium montazerii (=Serangium<br />
parcesetosum), 15<br />
Serratia marcescens, 257<br />
Services, 5<br />
Sesbania extract, 154<br />
Sesquiterpene hydrocarbons, 92<br />
Sesquiterpene, 199<br />
Setae, 239
360<br />
INDEX<br />
Sethoxydim, 137, 144, 152<br />
Seville orange, 3<br />
Sex allocation, 317, 324<br />
Sex pheromone, 48<br />
Sex pheromone-baited traps, 14<br />
Sex ratio, 81, 211, 220, 224, 296,<br />
300, 316, 317<br />
Sexual attractants, 6<br />
Shaddock, 3<br />
Shade tree, 133, 158<br />
Shelter, 222, 228<br />
Shield, 75, 79<br />
Shoot tips, 203<br />
Shoots, 94<br />
Shrubs, 238<br />
Shuckworm, 138, 139, 140<br />
Sicily, 15, 16, 18, 19, 78, 82, 84, 86,<br />
95, 96, 98, 99<br />
Sida rhombifolia, 143<br />
Side effects, 3, 21<br />
Sieving, 121<br />
Siglure, 92<br />
Signalling, 189–191, 195, 198–200,<br />
201–205<br />
Silk gl<strong>and</strong>s, 277<br />
Silk, 80, 277<br />
Simazine, 144<br />
Singapore, 239, 245<br />
Skin, 236, 239<br />
Skis, 134<br />
Slime, 273<br />
Slug, 122<br />
Soft scales, 13, 14, 17<br />
Software, 164, 169, 170, 171<br />
Soil bacteria, 240<br />
Soil chemicals, 114, 119<br />
Soil cylinders, 116<br />
Soil erosion, 147, 149, 150, 163<br />
Soil food webs, 101, 103, 111<br />
Soil micro<strong>org</strong>anisms, 150<br />
Soil mulches, 113<br />
Soil particles, 149<br />
Soil pH, 151<br />
Soil properties, 110, 114<br />
Soil texture, 107, 109, 114, 128<br />
Soil Treatments, 228<br />
Soil, 101, 103–105, 107, 109–116,<br />
119–120, 123–128, 209, 211, 214,<br />
216, 219, 224, 225–230<br />
Soilborne biological control agents, 107<br />
Soilborne <strong>org</strong>anisms, 116, 117<br />
Soil-inhabiting insects, 230<br />
Solanaceae, 320, 323<br />
Solanum, 143<br />
Solar radiation, 165<br />
Soldier beetles, 148<br />
Solenopsis invicta, 154, 161<br />
Solidago canadensis, 197<br />
Sonchus, 84<br />
Sooty mould, 13, 46, 87, 93<br />
S<strong>org</strong>hum, 155<br />
Sour orange, 3, 22<br />
South Africa, 64, 66, 68, 71, 83<br />
South America, 89, 93<br />
South Asian Tsunami, 164<br />
South-Eastern Asia, 75<br />
Soybeans, 155<br />
Space shuttles, 167<br />
Spain, 3–7, 12, 15–21, 23, 24, 26, 27,<br />
61–64, 69–71, 74, 81–84, 99, 101,<br />
109, 114, 115, 123, 124, 209–211,<br />
232<br />
Spatial resolution, 167<br />
Specialist phytoseiids, 317<br />
Specificity, 116, 118, 129<br />
Spectral ranges, 166<br />
Spectral resolution, 167<br />
Spectral signature, 165<br />
Speed, 240<br />
Sperchon, 288, 304<br />
Sperchontidae, 288<br />
Sphaerophoria, 46<br />
Sphyrapicus varius, 134<br />
Spider mite, 201, 267, 268, 269, 280,<br />
285, 297, 299, 301, 317, 320, 324,<br />
325<br />
Spider, 62, 66, 70, 81<br />
Spine, 80<br />
Spinning disc, 240<br />
Spinosad, 21, 22, 24, 25, 67, 68, 92<br />
Spiracles, 79<br />
Spirodiclofen, 22, 24
INDEX<br />
361<br />
Spiroplasma poulsonii, 260<br />
Spiroplasma, 257, 260, 300, 303<br />
Spiroplasmataceae, 260<br />
Spodoptera eridania, 196, 205<br />
Spodoptera exigua, 198, 199, 207<br />
Spodoptera frugiperda, 199<br />
Spodoptera littoralis, 109<br />
Sporangiophore, 261<br />
Sporangiospores, 261<br />
Spore, 112, 240, 241, 246, 254,<br />
260–264, 270–273, 277–279,<br />
283–286, 291–293, 296–299<br />
Sporothrix, 296<br />
Sporozoa, 286, 306<br />
Sporozoites, 290<br />
Sporting goods, 134<br />
Sporulation, 263, 268, 272, 297,<br />
299<br />
Spot treatment, 138<br />
SPOT VEG, 168<br />
SPOT-2, 168<br />
SPOT-4, 168<br />
SPOT-5, 168<br />
SPOT-VGT, 175<br />
Spray applications, 35, 36<br />
Spray program, 35, 142<br />
Spray treatments, 48<br />
Sprayers, 34, 141, 150<br />
Spraying, 34–36, 52, 197, 209, 211,<br />
216, 223, 227, 228, 240, 241, 245,<br />
251, 284<br />
Sprays, 34, 35, 39, 133, 136–139,<br />
141, 142, 152, 154–156, 252, 307<br />
Spring, 13, 14, 237, 241, 242<br />
Spurges, 143<br />
Squirrels, 134<br />
St<strong>and</strong>ard curve, 117<br />
St<strong>and</strong>ards, 5, 26<br />
Staphylinidae, 70, 72, 92<br />
Starvation, 255<br />
Starving mites, 255<br />
Steganacarus striculus, 288<br />
Steinernema abbasi, 216, 225, 226,<br />
229, 230<br />
Steinernema affine, 122<br />
Steinernema arenarium, 118<br />
Steinernema boemarei, 118<br />
Steinernema carpocapsae, 106, 224,<br />
225, 226, 229<br />
Steinernema cubanum, 118<br />
Steinernema diaprepesi, 109, 111,<br />
112, 117<br />
Steinernema glaseri, 109, 112, 118<br />
Steinernema gu<strong>and</strong>ongense, 118<br />
Steinernema kraussei, 122<br />
Steinernema longicaudum, 118<br />
Steinernema riobrave, 106, 109, 110,<br />
112<br />
Steinernema riobravis, 106, 224,<br />
226–229<br />
Steinernema scapterisci, 106<br />
Steinernema, 105, 110, 113, 113,<br />
117, 123–125, 127–129, 216,<br />
224–226, 229, 230<br />
Steinernematidae, 224<br />
Steinernematids, 111, 112<br />
Steneotarsonemus fragariae, 275<br />
Sterile insect technique, 32, 34<br />
Sticky cards, 77<br />
Sticky tape, 79<br />
Stigmella aurella, 84<br />
Stigmella, 83<br />
Stimuli, 33<br />
Stongylida, 112<br />
Storage, 270<br />
Stress factors, 312<br />
Strobilurins, 141<br />
Subsistence agriculture, 312<br />
Substrate, 321<br />
Sucrose centrifugation, 119<br />
Suction traps, 14<br />
Sudan, 173, 174, 176, 187, 188<br />
Sugarcane, 104, 124, 125, 218<br />
Suitable environments, 312<br />
Sulfur ammonium, 33<br />
Sulphur, 136, 294<br />
Sultanate of Oman, 209, 224, 225,<br />
230, 231<br />
Summary maps, 165<br />
Summer oils, 44<br />
Summer, 13, 237, 241<br />
Sunflower, 155
362<br />
INDEX<br />
Sunlight, 39, 90, 167, 251, 297<br />
Sunrise, 214<br />
Sunset, 214<br />
Surface water, 5<br />
Surveys, 164, 165, 171, 175, 176,<br />
178, 179, 186<br />
Survivability, 292<br />
Sustainable control, 36<br />
Swazil<strong>and</strong>, 83<br />
Sweet orange, 34, 73<br />
Switzerl<strong>and</strong>, 267<br />
Syagrus romanzoffiana, 284<br />
SYBR Green, 116, 127<br />
Symbionts, 249, 260, 296, 302, 303<br />
Symbiosis, 113<br />
Symbiotic entomopathogenic<br />
bacteria, 105<br />
Sympherobius, 87<br />
Sympodal conidiogenesis, 296<br />
Symptoms, 251, 253, 285<br />
Synergies, 312<br />
Synthetic fertilizers, 149<br />
Syria, 82, 84<br />
Syrphidae, 46<br />
Syrphids, 67<br />
Syrphophagus aphidivorus, 46<br />
Syrphus latefasciatus, 46<br />
Systemic expression, 191<br />
Systemic insecticides, 139<br />
T<br />
Taiwan, 82, 83, 168<br />
Tangerine, 3, 22<br />
Tape worm, 290<br />
Tapinoma nigerrimum, 11, 89<br />
Tapinoma simrothi, 11<br />
TaqMan, 118, 122<br />
Tarichium acaricolum, 266<br />
Tarichium azygosporicum, 266<br />
Tarichium distinctum, 266<br />
Tarichium hyalinum, 266<br />
Tarichium monokaryoticum, 266<br />
Tarichium obtusoangulatum, 267<br />
Tarichium pusillum, 267<br />
Tarichium sphaericum, 267<br />
Tarichium subglobosum, 267<br />
Tarichium svalbardense, 267<br />
Tarichium tenuisculpturatum, 267<br />
Tarichium uropodinis, 267<br />
Tarichium verruculosum, 267<br />
Tarichium, 262, 296<br />
Tarsonemidae, 12, 274, 275, 276,<br />
280, 283, 305, 306<br />
Tarsonemus lacustris, 276<br />
Tarsonemus, 274<br />
Tau-fluvalinate, 21, 22, 23, 26<br />
Taxon, 285<br />
Tebufenozide, 21, 22, 24, 26, 45, 139<br />
Tebufenpyrad, 21, 22, 24, 26, 53, 68<br />
Tectocepheus velatus, 266<br />
Tegumentary appendages, 236<br />
Teleomorphs, 272<br />
TEM, 252<br />
Temperature, 65, 78, 79, 81, 82, 88,<br />
90–91, 95, 110, 120, 140, 159,<br />
164, 169, 176, 209, 230, 237, 251,<br />
268, 270, 283, 294, 297, 306, 309,<br />
316, 325<br />
Temporal resolution, 168<br />
Tenuipalpidae, 12<br />
Tephritidae, 11, 24, 29, 62<br />
Terpenoid, 191, 200, 208<br />
TERRA/MODIS, 168<br />
Terrestrial traps, 219<br />
Tetranychidae, 12, 29–30, 50, 54,<br />
61, 66, 68, 70, 71, 72, 256, 257,<br />
264–266, 274, 276, 281, 300–305,<br />
307, 308<br />
Tetranychids, 50, 51, 53, 249, 252,<br />
297, 307, 316<br />
Tetranychus bimaculatus, 265<br />
Tetranychus cinnabarinus, 274, 276,<br />
280<br />
Tetranychus desertorum, 264<br />
Tetranychus evansi, 265, 284, 301, 305<br />
Tetranychus kanzawai, 256, 303<br />
Tetranychus ludeni, 266, 267<br />
Tetranychus neocaledonicus, 257<br />
Tetranychus pacificus, 254, 265, 303<br />
Tetranychus quercivorus, 257, 303<br />
Tetranychus truncates, 284<br />
Tetranychus tumidis, 267
INDEX<br />
363<br />
Tetranychus tumidus, 265, 268<br />
Tetranychus turkestani, 257, 265, 276<br />
Tetranychus urticae, 12, 13, 24, 29–30,<br />
50, 51, 57, 62, 63, 65, 66, 68, 69, 70,<br />
72, 75, 200, 201, 252, 254–257, 259,<br />
264–268, 274, 276, 280, 283–285,<br />
300, 302, 303, 305, 307, 308<br />
Tetranychus yusti, 256<br />
Tetrapolypus rhynchophori, 215<br />
Tetrastichus ceroplastae, 38<br />
Tetrastichus giffardianus, 20, 63<br />
Tettigonidae, 7<br />
Texas, 82, 104, 124, 136, 137, 140,<br />
156, 158, 159, 160, 267<br />
Thail<strong>and</strong>, 82, 83, 98<br />
ThaiPhat, 168<br />
Thaumetopoea pityocampa, 237, 238<br />
Thaumetopoea processioneae, 237<br />
Thaumetopoea wilkinsonii, 243<br />
Thaumetopoea, 237, 238, 243, 244,<br />
245, 246<br />
Thaumetopoeidae, 236, 237, 239,<br />
243–245<br />
The Netherl<strong>and</strong>s, 249, 253, 271, 292,<br />
303, 306–308<br />
Thelohania microtritiae, 289<br />
Thelytokous, 259<br />
Thelytoky, 259, 303<br />
Theoretical approaches, 314<br />
Thiamethoxam, 22, 23, 24, 47<br />
Thiophanate methyl, 141<br />
Thorax, 89, 220<br />
Threshold cycle, 116<br />
Thrip, 49<br />
Thripidae, 7<br />
Thrips australis, 7<br />
Thrips flavus, 7<br />
Thrips major, 7<br />
Thrips tabaci, 7, 292<br />
Thrips, 7, 23, 29–31, 49, 50, 54, 57<br />
Thuringiensin, 254, 255, 303, 307<br />
Thyme, 92<br />
Thysanoptera, 7, 23<br />
Ticks, 258, 303, 305, 307<br />
TMA, 32, 36<br />
Tobacco, 191, 195, 197<br />
Toddy palm, 209<br />
Tolypocladium, 296<br />
Tomato, 197, 198, 199, 201, 205,<br />
207, 320, 323<br />
Tool h<strong>and</strong>les, 134<br />
Topography, 164, 176<br />
TopSat, 168<br />
Tortricidae, 10, 30<br />
Toxicity, 255, 303<br />
Toxin, 107, 191, 199, 239<br />
Toxoptera aurantii, 8, 23, 29, 45, 47,<br />
62, 94<br />
Toxoptera citricida, 6, 8, 23, 45<br />
Toxoptera citricidus, 74, 94 (see also:<br />
Toxoptera citricida)<br />
Trachyuropoda coccinea, 267, 276,<br />
300<br />
Trachyuropodidae, 267, 276<br />
Trajectory Model, 176<br />
Transcriptional regulation, 200<br />
Transgenic phytoseiids, 322<br />
Transmission electron microscopy,<br />
252<br />
Transmission, 252, 253, 255, 260,<br />
264, 292, 297, 303, 304, 306, 307<br />
Transovarial transmission, 291<br />
Trap crops, 138, 155<br />
Trap design, 218<br />
Trap networks, 35<br />
Trapping fungi, 119<br />
Trapping program, 211<br />
Trapping, 3, 6, 14, 30–33, 48, 58,<br />
221, 223, 231, 232, 233<br />
Traps, 14, 32–37, 39, 40, 46, 48, 50,<br />
55–56, 58, 77, 78, 79, 88, 92, 115,<br />
125, 129, 211, 214, 218–222, 224,<br />
228–230<br />
Treatment, 35, 36, 41, 47, 55, 57<br />
Tree damage, 104<br />
Tree dormancy, 149<br />
Tree phenology, 137<br />
Tree, 5, 12, 13, 14, 65, 69, 74, 76, 81,<br />
86, 88, 92–94, 102–104, 107, 235,<br />
237, 239, 244, 245, 279, 280, 308<br />
Trials, 242<br />
Trichilia cipo, 194
364<br />
INDEX<br />
Trichlorfon, 21, 22, 24, 26<br />
Trichlorphon, 216<br />
Trichodorus similis, 122<br />
Trichomes, 194, 203, 206<br />
Trichoplusia ni, 197<br />
Tricouropoda szczecinensis, 266<br />
Trimedlure, 14, 32, 33, 92<br />
Trimethylamine, 32<br />
Trioza erytreae, 6, 7<br />
Trioza obsoleta, 83<br />
Triozidae, 7<br />
Tristeza virus, 6<br />
Trombiculidae, 256, 265<br />
Trombidiidae, 284<br />
Trombidium gigas, 284<br />
Trophic cascade, 111, 123, 125<br />
Tropinota hirta, 11<br />
Tropinota squalida, 11<br />
Trumpet creeper, 143<br />
Trunk injection, 209, 230<br />
Trunk treatment, 138<br />
Trunk, 76, 79, 87, 88, 134, 135, 137,<br />
154, 157, 209, 210, 216–218,<br />
226–230<br />
Tsunami, 185<br />
Tube-like sacs, 260<br />
Tunisia, 4, 26, 82, 84<br />
Tunnels, 210, 218, 226, 227, 312<br />
Turkey oak leaves, 242<br />
Turkey oak, 238, 242<br />
Turkey, 4, 5, 7, 15–20, 81, 82, 84, 99<br />
Tuscany, 242<br />
Twigs, 13, 14, 76, 79<br />
Twospotted spider mite, 75, 254, 255,<br />
259, 260, 267, 283, 284, 301<br />
Tydeidae, 274, 276<br />
Tydeus californicus, 276<br />
Tydeus gloveri, 276, 307<br />
Type A <strong>org</strong>anisms, 258<br />
Type B <strong>org</strong>anisms, 258<br />
Typhlodromalus aripo, 319<br />
Typhlodromalus limonicus, 319<br />
Typhlodromalus manihoti, 319<br />
Typhlodromips newsami, 319<br />
Typhlodromips sessor, 319<br />
Typhlodromus (A.) doreenae, 318<br />
Typhlodromus (Anthoseius)<br />
caudiglans, 318<br />
Typhlodromus (T.) exhilaratus, 318<br />
Typhlodromus (T.) pyri, 318<br />
Typhlodromus (T.) rickeri, 318<br />
Typhlodromus athenas, 51<br />
Typhlodromus athiasae, 280<br />
Typhlodromus cryptus, 77<br />
Tyroglyphidae, 288, 291, 309<br />
Tyrophagus perniciosus, 264<br />
Tyrophagus putrescentiae, 280, 288,<br />
291, 304<br />
U<br />
UAE, 209, 210, 216, 219–220, 224,<br />
225, 230<br />
Ultrastructural morphology, 253<br />
Ultraviolet, 166<br />
Unaspis citri, 6, 10, 23<br />
Unaspis yanonensis, 10, 19, 74<br />
United Arab Emirates, 209, 231, 232,<br />
233<br />
United Kingdom, 237, 312<br />
United States, 133, 151, 156, 159,<br />
160, 161<br />
University of Amsterdam, 271<br />
Uraba lugens, 238, 240, 244<br />
Urban environments, 235, 236<br />
Urban parks, 235<br />
Urban programs, 242<br />
Uric acid, 294<br />
Urobovella, 274<br />
Uropoda minima, 267<br />
Uropodina, 274, 300<br />
Uropodoidea, 274<br />
Urtica, 84, 97<br />
Urticating, 235, 236, 237, 238, 239,<br />
240, 241<br />
Uruguay, 106<br />
US, 48, 133, 134, 135, 140, 143, 148,<br />
152<br />
USA, 163, 168, 176, 186, 240, 250,<br />
267, 278, 283<br />
Ustilaginomycetes, 285<br />
Ustilagomycetes, 285, 301<br />
Uzbekistan, 177, 178, 182, 186, 187
INDEX<br />
365<br />
V<br />
Valencia, 67, 68, 72, 83<br />
Valine, 194, 206<br />
Varieties, 73, 87, 91<br />
Varroa destructor, 253, 254, 302,<br />
304, 306<br />
Varroa jacobsoni, 253, 284, 297,<br />
304<br />
Varroa mite, 253, 284, 297<br />
Vasates destructor, 275<br />
Vasates mckenzie, 276<br />
Vatacarus ipoides, 256<br />
Vatacarus, 256, 265<br />
Vector, 6, 252, 290, 297, 304<br />
Vegetable gardens, 179<br />
Vegetables, 104<br />
Vegetation distribution, 166<br />
Vegetation, 189, 190<br />
Vegetative period, 42<br />
Veigaia, 267<br />
Veigaiidae, 267<br />
Veneer, 134<br />
Veneto, 15<br />
Venezuela, 82, 268, 269, 300<br />
Ventral coating, 75<br />
Ventriculus, 292<br />
Verbascum thapsus, 198<br />
Vertebrate host, 250<br />
Vertebrates, 252, 253, 257, 258, 262,<br />
289, 300<br />
Vertical transmission, 255, 291<br />
Vertically Looking RADAR, 175<br />
Verticillium lecanii, 298<br />
Verticillium, 296, 298<br />
Victoria, 179<br />
Vigna radiata, 199<br />
Villages, 165<br />
Vines, 143<br />
Vineyards, 179<br />
Virulence, 251, 279, 284, 290, 297, 298<br />
Virus inhibitors, 252<br />
Virus like diseases, 6<br />
Virus particles, 250, 251<br />
Virus recognition, 295<br />
Virus suspensions, 251<br />
Virus vector, 122<br />
Virus, 6, 209, 216, 232, 249, 250,<br />
251, 252, 253, 254, 295, 297, 306<br />
Virus-infected mites, 253<br />
VLR, 175<br />
Volatile chemicals, 189, 191, 203,<br />
204, 272<br />
Volatiles, 190–192, 195, 196, 199–202,<br />
204, 205, 207, 208, 255, 272<br />
Volicitin, 191, 199, 201, 207<br />
W<br />
Wall, 258, 262, 290, 292<br />
Walnut caterpillar, 134<br />
Walnut, 76<br />
Warm periods, 13<br />
Warm-blooded <strong>org</strong>anisms, 236<br />
Warning, 30, 33, 37<br />
Waste products, 294<br />
Water conservation mechanism, 192<br />
Water potential, 110, 113<br />
Watering, 314<br />
Wavelength, 172<br />
Webworm larvae, 194<br />
Weed competition, 144, 146, 147<br />
Weed control, 136<br />
Weed science, 133<br />
Weeding, 73<br />
Weeds, 69, 89<br />
Weevil abundance, 107<br />
Weevil control, 101, 103, 106<br />
Weevil, 101, 103–105, 109, 110, 125,<br />
130, 136, 139, 140, 154, 209–212,<br />
214, 216–219, 221, 222, 224, 225,<br />
228, 229, 232, 233<br />
West Africa, 173, 174<br />
West Nile virus, 252<br />
Western tent caterpillar, 194<br />
White oil, 39, 47, 53<br />
Whiteflies, 13, 14, 29, 30, 40, 41, 68, 74<br />
Whitetail deer, 151<br />
Wild plant, 202<br />
Wildfire, 164, 165, 166<br />
Wildlife, 146, 147, 151, 152, 156<br />
Wind speed, 240<br />
Windbreaks, 314<br />
Wings, 79, 80, 89
366<br />
INDEX<br />
Winter, 32, 51, 237, 241<br />
Wire screen, 228, 229<br />
Wolbachia, 256, 258, 259, 260, 296,<br />
300, 301, 303, 304, 308, 309<br />
Wolbachieae, 257<br />
Wood fibers, 217<br />
Wood, 134, 135, 217, 227, 237, 238,<br />
240, 242<br />
Wooden frame, 227, 229<br />
Woolly whitefly, 29, 30, 40, 41, 42<br />
World War II, 147<br />
Wounding, 191<br />
Wounds, 253<br />
Wyoming, 163, 171, 185, 186, 187<br />
X<br />
Xenillus tegeocranus, 288<br />
Xenorhabdus, 105, 113, 125, 224<br />
X-rays, 166<br />
Xylella fastidiosa, 141<br />
Xylocorus galactinus, 215, 233<br />
Y<br />
Yellow pecan aphid, 138, 139<br />
Yellow sticky traps, 14<br />
Yellow water-pan traps, 14<br />
Yellow-bellied sapsucker, 134<br />
Yemen, 173<br />
Yield losses, 31, 40<br />
Young leaves, 13<br />
Z<br />
Z-7-tetradecenal, 48<br />
Zeta-cypermethrin, 22, 23, 24<br />
Zonate leaf spot, 142<br />
Zoophthora radicans, 265<br />
Zoospore movement, 112<br />
Zoospores, 104, 112<br />
Zygomycetes, 261, 300, 302, 303,<br />
304, 306<br />
Zygomycota, 260, 261, 296<br />
Zygospores, 260, 296<br />
Zygote, 260, 290