Untitled - International Rice Research Institute
Untitled - International Rice Research Institute
Untitled - International Rice Research Institute
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Contents<br />
Foreword<br />
Preface<br />
v<br />
vi<br />
INTRODUCTION 1<br />
FUNCTIONS OF SEED HEALTH TESTING 3<br />
Cataloguing pathogens of crops 3<br />
Detection methods 3<br />
Post introduction measures 5<br />
THE MISSING LINK 6<br />
Epidemiology 6<br />
Disease and infection cycles 7<br />
Seed transmission 8<br />
Relationship between seedborne inoculum and 9<br />
disease development in the field<br />
Inoculum level and inoculum thresholds 9<br />
Risk analysis 10<br />
Microorganisms associated with seed 11<br />
SEED HEALTH MANAGEMENT FOR CROP PRODUCTION 12<br />
IDENTIFICATION OF FUNGI DETECTED ON RICE SEED 13<br />
Seedborne fungi causing foliage diseases in rice 14<br />
Alternaria padwickii 14<br />
Bipolaris oryzae 17<br />
Cercospora janseana 21<br />
Microdochium oryzae 24<br />
Pyricularia oryzae 27<br />
Seedborne fungi causing stem, leaf sheath, and root diseases in rice 31<br />
Fusarium moniliforme 31<br />
Sarocladium oryzae 35<br />
Seedborne fungi causing grain and infloresence diseases in rice 38<br />
Curvularia sp. 38<br />
Fusarium solani 42<br />
Nigrospora sp. 44<br />
Phoma sorghina 47<br />
Pinatubo oryzae 51<br />
Tilletia barclayana 53<br />
Other fungi detected on rice seeds 57<br />
Acremoniella atra 58<br />
Acremoniella verrucosa 58<br />
iii
Alternaria longissima 59<br />
Alternaria tenuissima 59<br />
Aspergillus clavatus 60<br />
Aspergillus flavus-oryzae 60<br />
Aspergillus niger 61<br />
Chaetomium globosum 61<br />
Cladosporium sp. 62<br />
Curvularia eragrostidis 62<br />
Dreclslera hawaiiensis 63<br />
Epicoccum purpurascens 63<br />
Fusarium avenaceum 64<br />
Fusarium equiseti 65<br />
Fusarium larvarum 66<br />
Fusarium nivale 66<br />
Fusarium semitectum 67<br />
Gilmaniella humicola 67<br />
Memnoniella sp. 68<br />
Microascus cirrosus 68<br />
Monodictys putredinis 69<br />
Myrothecium sp. 70<br />
Nakataea sigmoidea 70<br />
Nectria haematococca 71<br />
Papularia sphaerosperma 71<br />
Penicillium sp. 72<br />
Pestalotia sp. 73<br />
Phaeoseptoria sp. 74<br />
Phaeotrichoconis crotolariae 74<br />
Pithomyces sp. 75<br />
Pyrenochaeta sp. 75<br />
Rhizopus sp. 76<br />
Septogloeum sp. 76<br />
Sordaria fimicola 77<br />
Spinulospora pucciniiphila 77<br />
Sterigmatobotrys macrocarpa 78<br />
Taeniolina sp. 78<br />
Tetraploa aristata 79<br />
Trichoderma sp. 79<br />
Trichothecium sp. 81<br />
Tritirachium sp. 81<br />
Ulocladium botrytis 80<br />
REFERENCES 82<br />
iv
Introduction<br />
The purpose of seed health testing is to assure the<br />
safe movement of seed of different crops, for research<br />
or trade. It is premised on the hypothesis that<br />
many harmful organisms are carried by and moved<br />
together with the seed, and that these organisms have<br />
the potential to cause severe damage to crop production<br />
and crop seed for international trade once they<br />
are introduced. Seed health testing information reveals<br />
the organisms carried by the seed and the level<br />
of infection, or infestation, that will be introduced to<br />
another region or country. The information, although<br />
useful, does not indicate the importance of organisms<br />
carried by the seed. For most plant diseases, this information<br />
is not available. Such information comes<br />
from experiments or surveys under field conditions<br />
where the seed is grown.<br />
Seed health testing can also be a means of quality<br />
control to improve seeding stocks for crop production<br />
by farmers. It is also useful for seed certification<br />
used by seed growers and public seed suppliers to<br />
farmers. Seed health testing is often done in the context<br />
of seed movement or trade for phytosanitary<br />
certification to meet plant quarantine regulations. The<br />
testing information, however, can also be applied to<br />
improve farmers’seed stocks for planting for crop<br />
management. In developing countries where farmers<br />
have to save their own seed for planting, knowledge<br />
of seed health can be very important to crop and pest<br />
management. It is a service that agricultural extension<br />
could provide. Farmers can acquire this knowledge<br />
through training. Seed health testing applied to<br />
seed certification would establish the standard for<br />
quality control. When the seed is put on the market,<br />
pest incidence is minimized and productivity of crop<br />
varieties is enhanced.<br />
<strong>Rice</strong> seed, like seeds of other crops, carries<br />
many organisms. Among them, fungi, bacteria, and<br />
nematodes are the most commonly detected microorganisms.<br />
These seedborne organisms can be<br />
pathogens and saprophytes. Many of the bacteria or<br />
fungi carried by rice seed are potential biological<br />
control agents against other rice pathogens. Some of<br />
them also promote seed germination and seedling<br />
vigor. The ecological relationship between these beneficial<br />
microorganisms and the pathogens or between<br />
pathogenic forms and nonpathogenic forms on rice<br />
seed needs further investigation. Very little research<br />
on this subject is published in scientific literature.<br />
Seedborne pathogens often serve as barriers to<br />
seed movement. Misunderstanding often arises because<br />
of insufficient biological and epidemiological<br />
data to guide the development of plant quarantine<br />
regulations. In scientific literature, research on<br />
seedborne pathogens focuses on developing methods<br />
for accurate and reliable detection of pathogens on or<br />
in the seed. Many importing countries need seed<br />
health information to determine whether the seed<br />
carries targeted pathogens important to quarantine.<br />
Without epidemiological data on the disease that the<br />
pathogen causes, we cannot establish the standard<br />
and level of importance of the disease. We know<br />
very little about crop damage and yield losses caused<br />
by pathogens carried by seed. Equally lacking is information<br />
about disease establishment in the field<br />
and the effect of seedborne pathogens on crop production.<br />
Not every pathogen carried by rice seed, for<br />
instance, is transmitted to the field when the seed is<br />
grown. Transmission varies from one pathogen to<br />
another and the same pathogen may react differently<br />
when the seed is sown in different growth conditions.<br />
These are important topics for further research. In<br />
this publication, we provide information on fungi<br />
commonly detected from rice seed during routine<br />
seed health testing. We also review briefly the missing<br />
links in information on seedborne pathogens and<br />
the seed as a source of inoculum for disease development<br />
in the field.<br />
Microorganisms carried by seeds can be classified<br />
as pathogens, nonpathogens, and nonpathogens<br />
with biological control properties. From the viewpoint<br />
of plant quarantine regulations, seed-carried microorganisms<br />
can be distinguished into either “hazard” or<br />
“common organisms” (Kahn and Mathur 1999).<br />
“Hazard” organisms involve those pathogens that<br />
have never been introduced into an area and can<br />
cause serious damage to crop production. Information<br />
on the level of damage caused by seedborne<br />
pathogens is not always available. The quarantine<br />
decision is often conservative to avoid any untoward<br />
consequences. Whether serious crop damage or<br />
yield losses would occur is a matter of speculation<br />
and not necessarily based on experimental results,<br />
1
which take into account various production situations<br />
and ecology. In reality, it is not possible or desirable<br />
to obtain seed lots free from any organism (Mew<br />
1997).<br />
From a plant pathologist’s point of view, there<br />
are missing links in documented information on<br />
seedborne pathogens. McGee (1995) pointed out the<br />
need for accurate information on seed transmission<br />
of some key seedborne pathogens. We need to study<br />
the epidemiology of seedborne pathogens in relation<br />
to disease development in the field. We need yield<br />
loss data to estimate the risk of seedborne pathogens.<br />
Furthermore, we need to study the role of seed health<br />
testing to improve farmers’ pest management and<br />
crop production. To know whether common pathogens<br />
carried by the seed pose a threat to crop production,<br />
we need to understand disease epidemiology.<br />
Conventional seed health testing provides adequate<br />
information about the frequency of detection from the<br />
seed and levels of seed infection. We need to assess<br />
whether these pathogens, upon detection, could be<br />
transmitted to the field when the seed is sown and if<br />
the disease that develops causes damage or injury to<br />
effect yield loss. In scientific literature, this information<br />
is not readily available or it needs to be confirmed.<br />
Very little research has been done in this<br />
area. Because of the increasing concern about<br />
seedborne pathogens, we need to understand their<br />
epidemiology. The initial inoculum is the key to understanding<br />
what causes an epidemic in a plant quarantine<br />
context. The threshold inoculum carried by a<br />
seed lot has to be defined in terms of its effect on<br />
transmission and disease establishment. Detection<br />
methods and the potential role of nonpathogenic microorganisms,<br />
especially those possessing biological<br />
control properties, must be studied and taken into<br />
account.<br />
2
Functions of seed health testing<br />
Seed health testing is done to determine microbial<br />
infection or contamination for quarantine purposes<br />
(e.g., international seed exchange or movement). It<br />
identifies the cause of seed infection that affects the<br />
planting value of seed lots for seed certification by<br />
seed growers to supply seed to farmers. Seed testing<br />
affects policies on seed improvement, seed trade,<br />
and plant protection. Neergard (1979) brought out the<br />
importance of pathogens carried by seeds and the<br />
disease potential assigned to pathogens.<br />
Several routine activities are undertaken during<br />
seed health testing. These include dry seed inspection,<br />
the standard blotter test for seed infection and<br />
contamination, postentry planting for field inspection<br />
of undetected plant diseases of seedborne and seedcontaminated<br />
pathogens, and certification. In seed<br />
multiplication for export, crop inspection prior to seed<br />
harvest offers an additional means to link seedborne<br />
pathogens and diseases of mother plants. All these<br />
activities provide preventive measures to eliminate<br />
the introduction of undesirable pathogens into a region<br />
or country. Seed health testing offers a powerful<br />
tool for documenting microorganisms associated with<br />
seeds. Information on microorganisms, however,<br />
needs to be associated with a database on yield loss<br />
and information on pathogens that cause diseases.<br />
Catalouging pathogens of crops<br />
For rice, seed health testing has been done on more<br />
than 500,000 seed lots following <strong>International</strong> Seed<br />
Testing Association (ISTA) rules (1985). A total of<br />
more than 80 fungi were detected on rice seeds<br />
(Table 1). The detection frequency varied. About 20<br />
species of fungal pathogens were detected from rice<br />
seed at any one time. Not all of them cause notable<br />
diseases in the field and it was not ascertained<br />
whether diseases were all seed-transmitted and, if so,<br />
what their transmission efficiency was. The role of a<br />
rice seed in a fungus life cycle is not clear.<br />
Pyricularia oryzae, the rice blast pathogen, although<br />
considered a very important rice pathogen,<br />
has the lowest detection frequency. The level varied<br />
according to seed source. Except Fusarium<br />
moniliforme, the seedborne inoculum of the other<br />
pathogens may not serve as an important source of<br />
secondary inoculum in the field. The infection level<br />
of P. oryzae is likely to be higher in temperate or<br />
subtropical environments than in tropical environments.<br />
The data set provides insights into the occurrence<br />
of rice fungal pathogens. The detection frequency<br />
and infection level are very high for Alternaria<br />
padwickii (80–90%) (Fig. 1). In tropical Asia,<br />
stackburn, the disease it causes, is hardly observed in<br />
the field.<br />
Detection methods<br />
Many detection methods have been developed over<br />
the years for various seedborne pathogens. We found<br />
the blotter test to be a common but efficient method<br />
of detecting seedborne fungal pathogens in rice seed.<br />
Following ISTA rules, the method involves plating<br />
400 seeds on some layers of moistened filter paper.<br />
Below is a list of the different detection methods used<br />
in routine seed health testing. Descriptions of these<br />
methods can be found in the references listed (see<br />
page 82).<br />
Seed health testing procedures involve techniques<br />
such as<br />
• Direct examination of dry seeds<br />
• Examination of germinated seeds<br />
• Examination of organisms removed by washing<br />
• Examination after incubation (both blotter and<br />
agar plates)<br />
• Examination of growing plants (for example,<br />
the seedling symptom test)<br />
• Embryo count methods<br />
• Molecular and serological techniques<br />
Other methods include a selective medium for<br />
specific pathogens. With advances in molecular<br />
techniques, emphasis in fungal identification and<br />
taxonomy has changed from a morphological approach<br />
(for example, spore size and spore shape) to<br />
a more functional approach based on aspects of the<br />
life cycle, mechanisms of spore production and release,<br />
DNA relationships, and physiological attributes.<br />
DNA analysis techniques such as the polymerase<br />
chain reaction (PCR), and random amplified<br />
polymorphic DNA (RAPD) analysis are the most<br />
commonly used tools.<br />
These are powerful techniques for detecting and<br />
for establishing the relationship between the inocu-<br />
3
Table 1. Fungi detected on rice seeds, IRRI Seed Health Unit (SHU) data (1983-97).<br />
Species Incidence a Species Incidence<br />
Alternaria padwickii +++<br />
Bipolaris oryzae +++<br />
Curvularia lunata +++<br />
C. oryzae +++<br />
Fusarium semitectum +++<br />
F. moniliforme +++<br />
Microdochium oryzae +++<br />
Phoma spp. +++<br />
Sarocladium oryzae +++<br />
Alternaria longissima ++<br />
Aspergillus clavatus ++<br />
A. flavus-oryzae ++<br />
A. niger ++<br />
Curvularia affinis ++<br />
C. oryzae ++<br />
Cladosporium sp. ++<br />
Epicoccum purpurascens ++<br />
Nakataea sigmoidea ++<br />
Nigrospora oryzae ++<br />
Penicillium sp. ++<br />
Pinatubo oryzae ++<br />
Pithomyces maydicus ++<br />
Rhizopus sp. ++<br />
Tilletia barclayana ++<br />
Ustilaginoidea virens ++<br />
Acremoniella atra +<br />
Alternaria tenuissima +<br />
Annellophragmia sp. +<br />
Botrytis cinerea +<br />
Cephalosporium sp. +<br />
Cercospora janseana +<br />
Chaetomium globosum +<br />
Chramyphora sp. +<br />
Colletotrichum sp. +<br />
Corynespora sp. +<br />
Cunninghamella sp. +<br />
Curvularia cymbopogonis +<br />
C. eragrostidis +<br />
C. inaequalis<br />
C. intermedia +<br />
C. ovoidea +<br />
C. pallescens +<br />
C. stapeliae +<br />
Cylindrocarpon sp. +<br />
Darluca sp. +<br />
Diarimella setulosa +<br />
Diplodia sp. +<br />
Drechslera cynodontis +<br />
D. dematioideum +<br />
D. halodes +<br />
D. hawaiiensis +<br />
D. longistrata +<br />
D. maydis +<br />
D. rostrata +<br />
D. sacharri +<br />
D. sorokiniana +<br />
D. turcica +<br />
D. tetramera +<br />
D. victoriae +<br />
Fusarium avenaceum +<br />
F. decemcellulare +<br />
F. equiseti +<br />
F. fusarioides +<br />
F. graminearum +<br />
F. larvarum +<br />
F. longipes +<br />
F. nivale +<br />
F. solani +<br />
F. tumidum +<br />
Gilmaniella humicola +<br />
Graphium sp. +<br />
Leptoshaeria sacchari +<br />
Masoniomyces claviformis +<br />
Melanospora zamiae +<br />
Memnoniella sp. +<br />
Microascus cirrosus +<br />
Monodictys levis +<br />
M. putredinis +<br />
Nectria haematococca +<br />
Nigrospora sphaerica +<br />
Papularia sp. +<br />
Penicillifer pulcher +<br />
Periconia sp. +<br />
Pestalotia sp. +<br />
Phaeoseptoria sp. +<br />
Phaeotrichoconis crotolariae +<br />
Phyllosticta sp. +<br />
Phyllosticta glumarum +<br />
Pyrenochaeta oryzae +<br />
Pyricularia grisea +<br />
Septogloeum sp. +<br />
Septoria sp. +<br />
Sordaria fimicola +<br />
Spegazzinia deightonii +<br />
Spinulospora pucciniiphila +<br />
Stemphylium sp. +<br />
Sterigmatobotrys macrocarpa +<br />
Taeniolina sp. +<br />
Tetraploa aristata +<br />
Trichoderma sp. +<br />
Trichosporiella sp. +<br />
Trichothecium sp. +<br />
Trichosporiella sp. +<br />
Tritirachium sp. +<br />
Ulocladium sp. +<br />
Verticillium albo-atrum +<br />
a<br />
+++ = frequent, ++ = moderate, + = low.<br />
4
% infected seed lots<br />
100<br />
80<br />
60<br />
40<br />
20<br />
Alternaria padwickii<br />
Sarocladium oryzae<br />
Fusarium moniliforme<br />
Bipolaris oryzae<br />
Pyricularia grisea<br />
Tilletia barclayana<br />
0<br />
1989 1990 1991 1992 1993 1994 1995 1996 1997<br />
Year<br />
Fig. 1. Detection of common seedborne fungal pathogens of rice from exported seeds at IRRI, 1989-97.<br />
Table 2. Level of fungal pathogens detected from seeds, field observations on seed planted in the field after<br />
treatment, disease incidence, and level of fungal infection detected from harvested seeds (24 entries; 1996 dry<br />
season).<br />
Field inspection for disease<br />
Fungal pathogen RSHT a at receipt (%) Disease %<br />
Entries infected RSHT at harvest<br />
Alternaria padwickii 15.7 Stackburn 0 A. padwickii 10.7<br />
Curvularia spp. 5.4 Black kernel 0 Curvularia spp. 9.0<br />
Sarocladium oryzae 0.8 Sheath rot 2 (8.3%) S. oryzae 2.7<br />
Gerlachia oryzae 2.7 Leaf scald 2 (8.3%) G. oryzae 0.2<br />
Fusarium moniliforme 0.2 Bakanae 0 F. moniliforme 3.8<br />
Bipolaris oryzae 1.7 Brown spot 0 B. oryzae 0.4<br />
Pyricularia grisea 0 Blast 1 (4.1%) P. grisea 0<br />
Phoma sp. 1.6 Glume blight 0 Phoma sp. 4.6<br />
Tilletia barclayana 0.3 Kernel smut 0 T. barclayana 0<br />
Disease-free 19 entries (79%)<br />
a<br />
RSHT = routine seed health test. Seed treatment applied: hot water, 52–57°C for 15 min plus Benlate and Dithane M-45 at 0.1% by seed weight.<br />
lum of seedborne pathogens and diseases in the field.<br />
Postintroduction measures<br />
“Damage control” often refers to actions taken to<br />
minimize damage after it has happened. The concept<br />
can be applied to seedborne fungal pathogen management<br />
by relating it to postquarantine treatment.<br />
There is always concern that if a pathogen is unintentionally<br />
introduced into a country or region, it may<br />
cause potential damage to the crop. The entry of infected<br />
seeds when seed lots are brought into a country<br />
is unavoidable. However, it is still not clear<br />
whether the infected seed being introduced will begin<br />
an infection of the crop in the field. It is desirable to<br />
limit the probability of infection. Several<br />
postquarantine treatments can be applied to control<br />
such damage. Many of these postquarantine treatments<br />
provide measures to counteract the introduction<br />
of undesirable pathogens (Table 2).<br />
Seed health testing is important to assure the<br />
safe movement of seed on the one hand and to control<br />
the spread of seedborne diseases through seed<br />
movement on the other hand.<br />
Seed treatment and seed health testing to eliminate<br />
potential pathogens are damage control steps<br />
intended to avoid the introduction of key pathogens.<br />
Currently available information or control measures<br />
in place may not be adequate. Some control measures,<br />
such as seed treatment, successfully check the<br />
movement of pathogens from the seed.<br />
5
The missing link<br />
Epidemiology<br />
There is little doubt that many pathogens are<br />
seedborne. Questions arise, however, on whether the<br />
introduction of seedborne inoculum of these pathogens<br />
would lead to the establishment of a disease in<br />
the field or whether the field population of a fungal<br />
pathogen is derived from the seedborne inoculum.<br />
Pathogens of significance to quarantine suggest<br />
the potential of seed transmission. They also relate to<br />
the potential damage or yield loss caused by diseases<br />
derived from the seedborne inoculum of the pathogen.<br />
However, there is very little accurate information<br />
about yield loss caused by rice diseases, and<br />
diseases derived from seedborne inoculum. Yield<br />
loss caused by a pest outbreak or a disease epidemic<br />
is important in determining pathogens with quarantine<br />
significance. There are very few comprehensive<br />
studies or databases on yield losses caused by pests<br />
or pathogens in scientific literature. Studies conducted<br />
and documented by Savary et al (1996, 1997,<br />
1998, 2000a,b), Savary and Willocquet (1999), and<br />
Willocquet et al (1999a,b) are some of the most comprehensive<br />
ones on rice diseases. Using both survey<br />
and experimental data, they developed pest and<br />
pathogen profiles for different rice production situations<br />
(PS). Production situations refer to the set of<br />
environmental conditions—climatic, technical, social,<br />
economic, and biological—under which agricultural<br />
production takes place. These were then related<br />
to yield losses with individual pests and pathogens,<br />
and also pest and pathogen profiles.<br />
Savary et al (1996, 1997, 1998, 1999) believe<br />
that by using such a systems approach combined<br />
with different statistical analyses, all these factors<br />
could be captured by a limited number of variables,<br />
such as those that describe patterns of cropping practices,<br />
for example, method of crop establishment,<br />
amount of chemical fertilizer used, type of weed<br />
control, and rice cultivar type (with or without disease<br />
resistance). In reality, farmers’ practices are, to a<br />
large extent, reflections of, or adaptations to, social,<br />
physical, and biological environments. Injury profiles<br />
refer to the sequence of harmful organisms that may<br />
occur during the crop cycle. Many such organisms<br />
affect rice. The number of processes by which a pest<br />
or pathogen may affect rice, however, is limited to<br />
less than 10, and injuries are often associated with<br />
one another. On this basis, yield losses caused by<br />
individual injuries as well as by injury profiles establish<br />
the importance of rice pests and diseases in specific<br />
PS at the regional level (Savary et al 2000a,b).<br />
The database identified sheath blight caused by<br />
Rhizoctonia solani AG1 and brown spot caused by<br />
Bipolaris oryzae as the two most important diseases<br />
in rice in Asia, each responsible for 6% yield loss,<br />
whereas blast caused by Pyricularia grisea and bacterial<br />
blight caused by Xanthomonas oryzae pv.<br />
oryzae account for 1–3% and 0.1% yield losses, respectively.<br />
However, most rice cultivars planted by<br />
Asian farmers are resistant to these two diseases. If<br />
cultivars possess no resistance to these two diseases,<br />
yield losses are likely to be higher than current estimates.<br />
Other diseases, such as sheath rot, stem rot,<br />
and those known as sheath rot complex and grain<br />
discoloration (Cottyn et al 1996a,b), are responsible<br />
for rice yield losses ranging from 0.1% to 0.5%. All<br />
other diseases alone or in combination would not<br />
cause more than 0.5–1% yield losses based on estimates.<br />
Projected yield losses cause by various rice<br />
diseases under different production situations are<br />
given in Table 3.<br />
In seed health testing, detection frequency<br />
means the number of pathogens detected in a seed<br />
lot. Infection frequency refers to the number of seeds<br />
(based on 400 seeds tested) within a seed lot which<br />
are infected (Mew and Merca 1992) and is equivalent<br />
to the inoculum level. In the epidemiological<br />
sense, no information is available to correlate detection<br />
frequency and infection frequency to seed transmission<br />
and disease establishment in the field. Still,<br />
there are other questions related to seedborne pathogens<br />
that must be answered. In rice, in which most<br />
fungal pathogens can be seedborne, and for which<br />
current farmer cultural practices have done little to<br />
improve quality (a result of farm labor shortage and<br />
short turnaround time), what is introduced to the field<br />
with seeds when the rice crop is planted? In seed<br />
production fields, it is necessary to practice disease<br />
management to produce disease-free seed?<br />
6
Table 3. Pathogen profiles closely associated with rice production situations (PS) and potential yield losses caused<br />
by rice diseases (adapted and modified from Savary et al 1998, Savary and Willocquet 1999).<br />
PS1 PS2 PS3 PS4 PS5 PS6 Yield loss<br />
(%)<br />
Actual yield (t ha –1 ) 4.8 4.6 3.5 6.7 3.8 3.9<br />
Disease<br />
Blast a L L M M 1–3<br />
Bacterial blight L L L L L 0.2<br />
Bakanae VL 0.0<br />
Brown spot L L VH H H 6.6<br />
Sheath blight VH VH M VH H H 6.4<br />
Sheath rot complex M M H M 0.5<br />
Grain discoloration M M H M 0.1<br />
Characteristics of environments<br />
Mineral fertilizer m l l h m h<br />
Fallow period l l m s m s<br />
Drought stress l l h l h m<br />
Water stress l l l h h h<br />
Crop establishment tr tr tr ds ds ds<br />
Herbicide use m l l m l l<br />
Insecticide use m m m m m m<br />
Fungicide use l l l h h h<br />
Previous crop rice rice w/b w/b rice rice<br />
a<br />
In the surveys, rice varieties possessing resistance to blast and bacterial blight diseases. For characteristics of environments, m = moderate, h =<br />
high, l = low, tr = transplanted rice, ds = direct-seeded rice, s = short, w/b = wheat or barley. For diseases and grain discoloration, L = low, M = medium,<br />
H = high, VH = very high.<br />
Disease and infection cycles<br />
Figure 2 shows how seedborne inoculum reinfects<br />
the seed during the development of a disease epidemic:<br />
seedborne inoculum → disease establishment<br />
→ disease development in the field (infection cycle)<br />
→ crop damage or yield loss (effect of seedborne<br />
inoculum) → reinfection of infestation of seed (potential<br />
dissemination to other fields, regions, or countries).<br />
There is voluminous information on seedborne<br />
pathogens of various crops derived from routine seed<br />
health testing for either certification or issuance of<br />
phytosanitary certificates. Information on transmission<br />
of the pathogen from the infected or infested<br />
seed to disease development in the field is scarce.<br />
Various factors that affect the infection cycle are<br />
weather conditions, cropping practices, resistance or<br />
susceptibility of the variety, virulence of the pathogen,<br />
and amount of incoculum produced for secondary<br />
spread and efficiency of the inoculum.<br />
It is often assumed that, for a pathogen to be<br />
seedborne, it must be seed-transmitted. McGee<br />
(1995) indicated that in only very few seedborne<br />
pathogens is the transmission clearly established.<br />
When conditions in the nursery bed and the<br />
ecosystem where rice is grown re taken into account,<br />
there is inadequate documentation on plant<br />
quarantine to guide decision making. It is not<br />
known under what specific conditions seedborne<br />
pathogens are transmitted to the crop at the seedling<br />
stage. Blast caused by P. oryzae and bakanae<br />
caused by F. moniliforme, are two of the better<br />
known diseases (Ou 1985). Once a disease is established<br />
in a crop, its intensity will depend on factors<br />
that influence the infection cycle. Climatic<br />
conditions and crop management practices are<br />
crucial to disease development.<br />
In rice, the infection frequency of P. oryzae is<br />
very low, yet the disease potential under a conducive<br />
environment (e.g., upland, subtropical, and<br />
temperate) is very high. Once seedlings are infected<br />
from seedborne inoculum, even at a low<br />
infection rate, millions of conidia are produced for<br />
secondary infection. On the other hand, seedborne<br />
F. moniliforme often induces bakanae with only<br />
one cycle of infection. Therefore, the initial inocu-<br />
7
Seedborne<br />
inoculum<br />
Reinfection/<br />
infection of seed<br />
Transmission<br />
(Establishment)<br />
Infected<br />
seed<br />
Crop damage/<br />
Injury (Impact)<br />
Inoculum<br />
production<br />
Disease<br />
development<br />
Infection<br />
efficiency<br />
Climatic<br />
conditions<br />
Cropping<br />
environments<br />
Fig. 2. Diseases and infection cycles of a seedborne fungal disease and its effect.<br />
lum for F. moniliforme is important. Once the<br />
seedborne inoculum is minimized, the disease is<br />
likely to be controlled.<br />
Changes in crop cultivation methods and cultural<br />
practices affect seedborne diseases. In traditional<br />
methods of cultivation, rice seedlings are raised in a<br />
seedbed with a saturated water supply. Because of<br />
the reduction in arable land and the decreasing productivity<br />
of available agricultural land, new methods<br />
of cultivation are being developed. These new methods<br />
are conducive to the transmission and development<br />
of seedborne diseases previously considered<br />
minor.<br />
In epidemiological research, seed transmission<br />
and establishment of disease derived from seedborne<br />
inoculum should be considered. These data are essential<br />
for assessing the importance of seedborne<br />
pathogens.<br />
Seed transmission<br />
McGee (1995) indicated that one of the missing links<br />
in seed health testing is the lack of information on<br />
seed transmission. Based on postquarantine planting,<br />
one of the difficulties encountered is distinguishing<br />
between a disease that developed from inoculum<br />
derived from the seed and that from other sources.<br />
Polymerase chain reaction (PCR) DNA technology<br />
is useful in this regard. Based on DNA fingerprinting,<br />
patterns of a pathogen population can be distinguished<br />
from those of the pathogen manifesting a<br />
disease on the crop grown from the seed. This<br />
would establish the transmission of the seedborne<br />
inoculum and its relation to the disease on the crop<br />
in the field. In routine disease monitoring of field<br />
crops such as rice or other nursery crops, identifying<br />
disease foci in nursery beds may be an alternative.<br />
For rice, this appears feasible at the seedling<br />
stage in the seedbed. A disease focus is a patch of<br />
crop with disease limited in space and time<br />
(Zadoks and van den Bosch 1994) and is likely to<br />
have been caused by the initial source of inoculum.<br />
In Japan, the seedbox nursery for rice provides an<br />
ideal means to identify the disease foci of single or<br />
different seedborne pathogens. The paper towel<br />
method, a very common method for testing seed<br />
germination, resulted in more seedling mortality<br />
and thus less germination than the seedbed method<br />
(seedbed with field soil) used in crop production<br />
(Table 4). The method used for assessing the effect<br />
of seedborne fungal pathogens on seed germination<br />
varies.<br />
8
Table 4. Germination (%) of untreated and treated seeds using paper towel and in-soil germination methods (400<br />
seeds each; randomized complete block design).<br />
Normal a Abnormal Dead seeds<br />
Varieties Paper In-soil Paper In-soil Paper In-soil<br />
towel test towel test towel test<br />
Untreated<br />
IR62 79.7 ab 91.7 a 16.0 a 5.3 a 4.3 a 3.0 b<br />
SARBON 65.3 b 75.7 ab 20.3 a 12.0 a 14.3 a 12.3 ab<br />
C22 94.0 a 84.0 ab 4.3 b 10.3 a 1.7 a 5.7 ab<br />
BS1-10 68.0 b 72.7 b 18.3 a 11.0 a 13.7 a 16.3 a<br />
Hot-water treatment<br />
IR62 86.7 a 85.3 a 5.0 b 7.7 b 8.3 b 7.0 b<br />
SARBON 46.3 b 50.3 c 19.7 a 10.3 b 34.0 a 39.3 a<br />
C22 92.3 a 94.3 a 5.0 b 4.0 b 2.7 b 1.7 b<br />
BS1-10 76.3 a 67.7 b 13.7 ab 25.0 a 10.0 a 7.3 b<br />
a<br />
In a column under each treatment, means followed by a common letter are not significantly different at the 5% level by Duncan’s multiple range<br />
test.<br />
Relationship between seedborne inoculum<br />
and disease development in the field<br />
In determining the importance of a seedborne pathogen,<br />
it is essential to relate inoculum production and<br />
the efficiency of the secondary spread to the inoculum<br />
threshold and disease severity after establishment.<br />
For a monocyclic disease, initial infection<br />
should be closely related to the initial inoculum provided<br />
by the seed. For a polycyclic disease, a low<br />
level of seedborne inoculum is adequate to begin<br />
infection from the seedbed to the main field, and increase<br />
disease intensity if climatic or crop-growing<br />
conditions are favorable. For instance, in rice blast<br />
caused by P. oryzae with low detection and infection<br />
frequencies, seed-carried inoculum is more important<br />
in temperate or subtropical environments than in<br />
a tropical lowland environment. In the former environments,<br />
the likelihood of seed-carried inoculum<br />
beginning an infection and producing a sufficient<br />
amount of inoculum for secondary infection is higher<br />
(Ou 1985).<br />
Inoculum level and inoculum thresholds<br />
In seed health testing for certification, the inoculum<br />
threshold of seedborne pathogens is defined as the<br />
amount of seed infection or infestation that can cause<br />
a disease in the field under conducive conditions and<br />
lead to economic losses (Kuan 1988). We believe<br />
that this should mean a minimal amount of seed infection<br />
or infestation. In principle and as Gabrielson<br />
(1988) indicated, one infected seed may give rise to<br />
one infected plant, but, under field conditions, this is<br />
hardly the case. The values of the inoculum threshold<br />
for different crop-pathogen combinations in different<br />
countries vary widely (Gabrielson 1988).<br />
Our experience with rice has shown that the<br />
potential of a seedborne pathogen to cause a disease<br />
is determined by the type of pathogen in relation to<br />
the crop growth environment. Under conditions in a<br />
wet-bed nursery for rice seedlings, the likelihood of a<br />
fungal pathogen beginning an infection appears less<br />
than under tropical conditions. Perhaps this is because<br />
of the microbial competition or antagonism.<br />
On the other hand, if the level of seedborne inoculum<br />
is high (we have not had it quantified), then the probability<br />
of it causing infection is also high. As one infected<br />
seed begins one disease focus and this focal<br />
point expands, the probability of infection increases.<br />
In reality, disease establishment is affected by inoculum<br />
density and the crop cultivation environment.<br />
The more infected seeds there are (inoculum level),<br />
the higher the probability of having an infection.<br />
We have monitored detection levels of seedborne<br />
fungal pathogens from imported seed lots by<br />
planting them in the field after seed treatment for<br />
postentry plant quarantine observation. Diseases observed<br />
were not related to seedborne pathogens<br />
(Table 2). Pathogens from harvested seeds from<br />
these plants were detected, but we are not sure<br />
whether these fungal pathogen populations were the<br />
same as those carried by the original seed or if they<br />
came from other sources in the field.<br />
9
For other fungal pathogens, there is a close relation<br />
between seed infection and infected plants<br />
grown from these seeds. An example is blackleg of<br />
crucifer caused by Phoma lingam (Leptosphaeria<br />
maculans) (Gabrielson1983). The classical example<br />
from Heald (1921) indicated that the sporeload of<br />
seeds was highly correlated to the percentage of<br />
smut appearing in the field.<br />
Inoculum thresholds vary according to cultural<br />
environments. In Japan, for instance, after rice cultivation<br />
became mechanized and seedlings were<br />
raised indoors in seedboxes, the occurrence of many<br />
seedborne fungal and bacterial pathogens increased.<br />
This is because the indoor conditions—high temperature<br />
and high humidity with artificial light—are very<br />
favorable for seedling disease development. As a<br />
result, the inoculum threshold is lower than that of<br />
seedlings raised outdoors under a field nursery. The<br />
inoculum becomes more efficient under certain conditions.<br />
Inoculum efficiency is determined by various<br />
factors. The type of disease and crop-growing environments<br />
are important. Gabrielson (1988) cautioned<br />
that thresholds must be developed for average environmental<br />
conditions of crop growth because they<br />
are influenced by all factors affecting the epidemiology<br />
of each host-parasite combination. It is difficult<br />
to use a single threshold of a single disease for all<br />
cropping environments. There is no clear definition<br />
on levels of threshold for the different pathogens detected<br />
from the seed. In rice, different fungal pathogens<br />
are detected from the seed (Table 1) and all of<br />
them are distributed throughout the rice-growing<br />
countries worldwide. Disease potential, however,<br />
depends on the rice ecosystem (upland, rainfed, irrigated,<br />
tropical, subtropical, and temperate environments,<br />
and deepwater and tidal coastal areas), cultural<br />
conditions, and types of crop management and<br />
production. Whether there is a need to treat all diseases<br />
the same way or differently for different ecosystems<br />
and production levels needs careful study.<br />
There is a general agreement that the threshold level<br />
for a disease is zero in an area if it has not been reported<br />
there.<br />
Risk analysis<br />
Risk analysis should serve an important basis for<br />
developing plant quarantine regulations. Risk analysis<br />
based on seed health testing needs to consider the<br />
following factors:<br />
1. type of pathogens<br />
2. role of seed in the life cycle of the<br />
pathogen<br />
3. disease or epidemic potential<br />
4. genetic variability of the pathogen<br />
5. type or site of initial infection<br />
6. kind of crop production environment (Mew<br />
1997)<br />
The risk of infection from seedborne pathogens<br />
is a function of risk probability and risk magnitude.<br />
Furthermore, risk probability is determined by introduction<br />
risk, that is, the probability that a pathogen<br />
enters a region or a field through the seed, the epidemiological<br />
risk, the probability that the pathogen establishes<br />
infection through seedborne inoculum. Risk<br />
magnitude is the potential consequence of an epidemic<br />
caused by the pathogen. Consequences are<br />
considered from the viewpoint of yield loss. Seed<br />
health testing results provide actual data on a pathogen<br />
that could potentially be introduced into a region<br />
or a field. The risk magnitude can be computed from<br />
a yield loss database or from modeling. In rice, this<br />
kind of database is available at IRRI. The yield loss<br />
database provides an estimate of losses and “hazards”<br />
caused by a pathogen once the infection is established<br />
through seedborne inoculum.<br />
However, data are lacking on the transmission<br />
efficiency of seedborne inoculum of many rice<br />
seedborne pathogens. A concerted effort is needed to<br />
compile this information through international collaboration.<br />
<strong>Research</strong> on seed pathology provides the<br />
basis for setting seed health testing policy, while information<br />
on pest or pathogen risk provides a starting<br />
point for seed health testing on target organisms for<br />
plant quarantine regulations. Very limited or no financial<br />
support is available for this important area of<br />
activities.<br />
A yield loss database can estimate the “hazards”<br />
of a pathogen once an infection is established<br />
through the introduction of a seedborne inoculum.<br />
However, data on inoculum levels and thresholds are<br />
also needed to develop realistic assessment or measurement<br />
procedures for some important seedborne<br />
pathogens. Data on seed transmission of many<br />
pathogens and transmission efficiency of seedborne<br />
inoculum are currently not available.<br />
Although conventional seed health testing provides<br />
adequate information on detection frequency<br />
and infection levels of some pathogens, we need to<br />
assess whether these pathogens cause any real injury<br />
to effect yield loss. In scientific literature, this information<br />
is not readily available.<br />
10
Microorganisms associated with seed<br />
Not all microorganisms associated with seed are<br />
pathogens. Some microorganisms possess biological<br />
control properties. The occurrence of nonpathogenic<br />
Xanthomonas has further complicated the issue of<br />
seedborne bacterial pathogens. Cottyn et al (2001)<br />
and Xie et al (2001) proved that seedborne antagonistic<br />
bacteria are present in rice and promote seed germination<br />
and seedling vigor, and also suppress disease<br />
with an inoculum from the seed. Microflora<br />
associated with the seed may be roughly categorized<br />
into pathogens and nonpathogens. The study by<br />
Cottyn et al (2001), supported by the Belgium<br />
Adminstration for Development Cooperation, and<br />
Xie et al (2001) showed that rice seed carries many<br />
bacteria belonging to 17 genera and over hundreds of<br />
species. Predominant were Enterobacteriacae<br />
(25%), Bacillus spp. (22%) and Pseudomonas spp.<br />
(14%). Other bacteria regularly present were<br />
Xanthomonas spp., Cellulomonas flavigena, and<br />
Clavibacter michiganense. We found that about 4%<br />
of the total bacterial population possesses biological<br />
control properties against most seedborne pathogens.<br />
Also, seedling vigor was enhanced after soaking<br />
seeds in bacterial suspension. These studies show<br />
that rice seed not only carries pathogens but also<br />
abundant microorganisms that act as biological control<br />
agents. Whether they play a bigger role in crop<br />
production and disease management needs further<br />
research. More support should be given to this research<br />
area, which is a vital part of a farmers’ internal<br />
resource management for sustainable crop production<br />
and disease management.<br />
11
Seed health management for crop production<br />
In tropical Asia, the productivity of newly released<br />
modern rice cultivars declines rapidly because of<br />
seed health problems associated with the continuous<br />
use of the seed without adequate seed health management.<br />
At IRRI, we have conducted research on<br />
seed health management since the early 1990s. The<br />
research effort has focused on understanding farmers’<br />
seed health problems in relation to crop management<br />
and production. By improving farmers’ seed<br />
health management, rice yield could be increased by<br />
5–20%. Increasing farmers’ yields generates more<br />
income and profit. The marginal cost-benefit ratio<br />
was estimated at 5, and even 10, depending on the<br />
quality of the farmers’ original seed stock for planting<br />
(T.W., unpubl. data).<br />
Seed health management is an important way of<br />
reducing pest damage and weed infestation in the<br />
field. By employing sound seed health management,<br />
farmers not only minimize the use of harmful agrochemicals,<br />
they also maximize the genetic yield potential<br />
of these modern rice cultivars. We found that<br />
the productivity of foundation seed is reduced by 1 t<br />
ha –1 in three crop seasons using current farmers’<br />
seed health management practices (L. Diaz, M.<br />
Hossain, V. Merca, and T.W. Mew, unpubl. data).<br />
Yield changes according to the level of “high-quality<br />
seed” in seed stock used by farmers. When the level<br />
of high-quality seed reached 90% of the seed stock<br />
for planting, the yield increase was not significant.<br />
In rice seed health testing, little information exists<br />
on pathogen detection frequency on seed and on<br />
which part of the seed an organism is likely to be<br />
located. This handbbok contains information on rice<br />
seed health testing that we have been carrying out for<br />
the past 20 years. We hope to offer seed health testing<br />
technicians, college or graduate students, and<br />
teachers in plant pathology or seed technology a useful<br />
guide. Information on seed health testing can also<br />
be an important means of improving crop production<br />
practices of farmers. The information contained in<br />
this handbook is based on IRRI’s rice seed health<br />
testing activities on both incoming and outgoing<br />
seeds. Thus, the material provides a reference for<br />
many seed health testing laboratories. In view of the<br />
increasing interest in international trade in rice, the<br />
handbook also serves as a basis for establishing plant<br />
quarantine guidelines for individual countries.<br />
12
Identification of fungi detected on rice seed<br />
The standard detection method used in identifying<br />
fungi on rice seed at IRRI is given below. Figure 3<br />
shows the parts of a rice seed attacked by fungi.<br />
With this method, numerous fungi have been detected<br />
on rice seed. The profile of each fungus detected<br />
is presented in the following pages.<br />
Methods and conditions of rice seed incubation<br />
for microorganism detection are listed below.<br />
The <strong>International</strong> Rules for Seed Testing recommend<br />
the blotter test for detecting seedborne fungi.<br />
The procedure involves these steps:<br />
1. Prepare materials (9.5-cm plastic petri dish,<br />
marking pencil, round blotter paper, distilled<br />
water, sampling pan, forceps, seed sample).<br />
2. Label plates accordingly using a marking<br />
pencil.<br />
3. Place 2–3 pieces of moistened round blotter<br />
paper in labeled plastic petri dishes.<br />
4. Sow 25 seeds per plate making sure that<br />
seeds are sown equidistantly with 15 seeds on<br />
the outer ring, 9 seeds at the inner ring, and 1<br />
seed in the middle.<br />
5. Incubate seeded plates at 21 °C under a 12-h<br />
light and 12-h dark cycle. Light sources can<br />
be near ultraviolet (NUV) light or daylight<br />
fluorescent tubes. The NUV light source can<br />
be a 320–400 nm lamp, preferably Philips<br />
TLD 36W/08 or GE F 40 BL. Daylight fluorescent<br />
tubes can be Philips TL 40W/54 day<br />
light or its equivalent.<br />
6. Examine each of the seeds after 5–7 d of<br />
incubation for fungal growth.<br />
Partition between<br />
lemma and palea<br />
Lemma<br />
Awn<br />
Sterile lemmas<br />
Palea<br />
Fig. 3. Parts of a rice seed.<br />
13
Seedborne fungi causing foliage diseases in rice<br />
Alternaria padwickii (Ganguly) Ellis<br />
syn. Trichoconis padwickii Ganguly<br />
Trichoconiella padwickii (Ganguly) Jain<br />
Disease caused: stackburn<br />
a. Symptoms<br />
On leaves—large oval or circular spots with a<br />
pale brown center and distinct dark brown margin.<br />
Color of center eventually becomes white and<br />
bears minute black dots.<br />
On grains—pale brown to whitish spots with black<br />
dots at the center and dark brown border.<br />
Roots and coleoptile of germinating seedlings—<br />
dark brown to black spots that eventually coalesce.<br />
Small, discrete, and black bodies are<br />
formed on the surface of the darkened area as<br />
decay proceeds.<br />
b. Occurrence/distribution<br />
Stackburn disease is widespread in most of the<br />
rice-growing countries worldwide (Fig. 4).<br />
c. Disease history<br />
The disease was first reported in the U.S. It resembles<br />
black rust of wheat on rice leaves, but<br />
only sclerotia and mycelium were observed.<br />
Later the fungus was observed in and on rice<br />
seeds.<br />
d. Importance in crop production<br />
Stackburn leaf spot disease is not considered to<br />
be of economic importance. However, seed infection<br />
results in grain discoloration, which may<br />
reduce germination and lower grain quality. The<br />
disease potential of stackburn is very low and the<br />
yield loss caused by A. padwickii in literature<br />
may be overestimated. The effect of infected<br />
seed on seed germination is not yet properly assessed.<br />
Detection on seed<br />
a. Incubation period on blotter<br />
A. padwickii is easily observed on seeds using the<br />
blotter method 5 d after seeding on moistened<br />
blotter and incubated under NUV at 21 °C. The<br />
detection frequency is about 67.1% on seeds<br />
coming from different regions (Fig. 5a,b).<br />
b. Habit character<br />
Seed infected with A. padwickii after incubation<br />
shows abundant aerial mycelia, hairy to cottony,<br />
profusely branched, grayish or hyaline when<br />
Fig. 4. Occurence of stackburn (Ou 1985, Agarwal and Mathur 1988, EPPO 1997).<br />
14
Detection frequency (%)<br />
100<br />
80<br />
60<br />
40<br />
20<br />
0<br />
Detection level (%)<br />
100<br />
80<br />
East Asia<br />
Europe<br />
Latin America<br />
South Asia<br />
Southeast Asia<br />
Sub-Saharan Africa<br />
60<br />
40<br />
20<br />
0<br />
1990 1991 1992 1993 1994 1995 1996 1997<br />
Year<br />
Fig. 5. Detection level (a) and frequency (b) of Alternaria padwickii from imported untreated seeds, 1990-97.<br />
young, becoming creamy yellow when mature;<br />
pinkish to light violet pigmentation is produced on<br />
the blotter; conidia are borne singly per conidiophore;<br />
darker than mycelia; sterile appendage<br />
prominent (Fig. 6a-c).<br />
c. Location on the seed<br />
A. padwickii is most often observed growing over<br />
the entire seed surface (36%) (Fig. 7).<br />
Microscopic character<br />
a. Mycelia—septate, profusely branched; hyaline<br />
when young, becoming creamy yellow when mature;<br />
branches arising at right angles from the<br />
main axis (Fig. 6d).<br />
b. Conidiophore—simple, not sharply distinguishable<br />
from mature hyphae, often swollen at the apex,<br />
hyaline when young, becoming creamy yellow<br />
when mature (Fig. 6e).<br />
c. Conidia—straight, shape varies from fusiform to<br />
obclavate and rostrate or in some cases<br />
elongately fusoid; with long sterile appendage; at<br />
first hyaline, becoming straw-colored to golden<br />
brown; thick-walled; 3–5 septate; constricted at<br />
the septum; 4- to 5-celled, second cell from the<br />
base larger than the rest of the cells (Fig. 6f).<br />
Measurements: 81.42–225.40 µ long including<br />
appendage; 11.96–23.46 µ wide at the broadest<br />
part and 2.99–5.52 µ wide at the center of the appendage<br />
(PSA); 83.95–203.78 µ long including<br />
appendage; 9.66–17.48 µ wide in the broadest part<br />
and 3.45–5.75 µ wide at the middle of the appendage.<br />
Colony characters on culture media (Fig. 8)<br />
Colonies on potato dextrose agar (PDA) incubated at<br />
ambient room temperature (ART) (28–30 °C) grow<br />
15
→<br />
a<br />
b<br />
→<br />
e<br />
f<br />
→<br />
f<br />
→<br />
c<br />
d →<br />
→<br />
Fig. 6. Habit character of Alternaria padwickii (Ganguly) Ellis on (a) whole seed (8X) and on sterile lemmas at (b)<br />
12.5X and (c) 25X. Photomicrograph of A. padwickii showing (d) mycelia, (e) conidiophore, and (f) conidia at 40X<br />
and stained with lactophenol blue.<br />
Observed frequency (%)<br />
40<br />
30<br />
20<br />
10<br />
0<br />
Sterile<br />
lemmas<br />
Awn<br />
Partition<br />
bet. lemma<br />
and palea<br />
Seed part<br />
Entire<br />
seed<br />
Lemma/<br />
palea<br />
only or<br />
both<br />
Fig. 7. Observed frequency of Alternaria padwickii<br />
occurrence on seed part.<br />
Fig. 8. Plate culture of Alternaria padwickii Ellis showing<br />
colony growths on potato dextrose agar (PDA), potato<br />
sucrose agar (PSA), and malt extract agar (MEA)<br />
incubated at ambient room temperature (ART), 21 °C,<br />
and 28 °C at 15 d after inoculation.<br />
16
moderately fast and attain a 4.32-cm diam in 5 d.<br />
They are slightly zonated, thickly felted, and grayish,<br />
becoming light outward. On the reverse side of the<br />
agar plate, the colony is azonated, black, and lighter<br />
outward. At 21 °C under alternating 12-h NUV light<br />
and 12-h darkness, colonies grow moderately fast<br />
and attain a 4.14-cm diam in 5 d. They are azonated,<br />
becoming markedly zonated outward, felted, yellowish<br />
to greenish gray, with a 0.5-cm sterile white margin.<br />
On the reverse side of the agar plate, the colony<br />
appears zonated and black and light outward. At 28<br />
°C under alternating 12-h light and 12-h darkness,<br />
colonies grow moderately fast and attain a 4.33-cm<br />
diam in 5 d. They are zonated, felted, and greenish<br />
gray. On the reverse side of the agar plate, the colony<br />
is zonated and black and yellowish brown outward.<br />
Colonies on potato sucrose agar (PSA) incubated<br />
at ART (28–30 °C) grow moderately fast and<br />
attain a 4.18-cm diam in 5 d. They are deeply felted,<br />
zonated with an even margin, and gray. The colony<br />
appears zonated and black on the reverse side of the<br />
agar plate. At 21 °C under alternating 12-h NUV and<br />
12-h darkness, colonies grow moderately fast and<br />
attain a 4.36-cm diam in 5 d. They are slightly zonated<br />
with a light gray submerged advancing margin,<br />
felted, and dark greenish gray. The colony appears<br />
slightly zonated, black, and lighter outward on the<br />
reverse side of the agar plate. At 28 °C under alternating<br />
12-h light and 12-h darkness, colonies grow<br />
moderately fast and attain a 4.06-cm diam in 5 d.<br />
They are zonated, felted with a sinuate margin, yellowish<br />
to greenish gray, and lighter at the margins.<br />
The colony appears zonated and black, and yellowish<br />
brown outward on the reverse side of the agar<br />
plate.<br />
Colonies on malt extract agar (MEA) incubated<br />
at ART (28–30 °C) grow moderately fast and attain a<br />
4.53-cm diam in 5 d. They are zonated, felted, and<br />
light gray to gray. The colony appears zonated and<br />
black on the reverse side of the agar plate. At 21 °C<br />
under alternating 12-h NUV and 12-h darkness, colonies<br />
grow moderately fast and attain a 4.47-cm diam<br />
in 5 d. They are azonated, becoming markedly zonated<br />
outward, and white to yellowish gray and becoming<br />
gray outward. The colony appears zonated<br />
and black with a light gray margin on the reverse side<br />
of the agar plate. At 28 °C under alternating 12-h<br />
fluorescent light and 12-h darkness, colonies grow<br />
moderately fast and attain a 4.90-cm diam in 5 d.<br />
They are zonated, felted, and greenish gray, becoming<br />
gray at the margins. The colony appears slightly<br />
zonated and black on the reverse side of the agar<br />
plate.<br />
Bipolaris oryzae (Breda de Haan) Shoem.<br />
syn. Drechslera oryzae (Breda de Haan) Subram. & Jain<br />
Helminsthosporium oryzae<br />
teleomorph: Cochliobolus miyabeanus (Ito & Kurib)<br />
Disease caused: brown spot (brown leaf spot or<br />
sesame leaf spot)<br />
Helminsthosporium blight<br />
a. Symptoms<br />
On leaves—small and circular dark brown or<br />
purple brown spots eventually becoming oval<br />
(similar to size and shape of sesame seeds) and<br />
brown spots with gray to whitish centers, evenly<br />
distributed over the leaf surface; spots much<br />
larger on susceptible cultivars. A halo relating to<br />
toxin produced by the pathogen often surrounds<br />
the lesions.<br />
On glumes—black or brown spots covering the<br />
entire surface of the seed in severe cases. Under<br />
favorable environments, conidiophore and conidia<br />
may develop on the spots, giving a velvety appearance.<br />
Coleoptile—small, circular, or oval brown spots.<br />
b. Occurrence/distribution<br />
Brown spot is distributed worldwide and reported<br />
in all rice-growing countries in Asia, America,<br />
and Africa (Fig. 9). It is more prevalent in rainfed<br />
lowlands and uplands or under situations with abnormal<br />
or poor soil conditions.<br />
c. Disease history<br />
This fungus was first described in 1900 and<br />
named as Helminthosporium oryzae. In Japan, the<br />
teleomorph was found in culture and was named<br />
Ophiobolus miyabeanus. However, Drechsler<br />
decided it belonged to Cochliobolus and renamed<br />
17
Fig. 9. Occurrence of brown spot (Ou 1985, Agarwal and Mathur 1988, EPPO 1997).<br />
it Cochliobolus miyabeanus. Because of the bipolar<br />
germination of the conidia, the anamorph of C.<br />
miyabeanus was changed to Bipolaris oryzae.<br />
d. Importance in crop production<br />
Bipolaris oryzae causes seedling blight, necrotic<br />
spots on leaves and seeds, and also grain discoloration.<br />
Severely infected seeds may fail to germinate.<br />
Seedling blight is common on rice in both<br />
rainfed lowlands and uplands. Under these rice<br />
production situations, brown spot can be a serious<br />
disease causing considerable yield loss. In history,<br />
the Bengal famine of 1942 is attributed to brown<br />
spot.<br />
Detection on seed<br />
a. Incubation period on blotter<br />
B. oryzae is easily observed on seeds using the<br />
blotter method 5 d after seeding on moistened<br />
blotter incubated under NUV light at 22 °C. The<br />
detection frequency is about 56.7% on seeds coming<br />
from different regions (Fig. 10a,b).<br />
b. Habit character<br />
There are two types of fungal detection on rice<br />
seed: type I shows less conidia and abundant<br />
aerial mycelia, fluffy to cottony; gray, greenish<br />
gray to black; conidiophores are usually slender<br />
and hard to distinguish from main mycelia;<br />
conidia are darker than mycelia, borne singly on<br />
the terminal portion of the hyphae.<br />
Type II shows abundant conidia and aerial<br />
mycelia are either absent or scanty. Conidiophores<br />
are straight or flexuous, relatively long;<br />
simple, brown to dark brown, arising directly from<br />
seed surface either solitary or in small groups<br />
bearing conidia at the end and/or on the sides,<br />
usually with 3–5 conidia per conidiophore (Fig.<br />
11a-c).<br />
c. Location on seed<br />
B. oryzae is often observed on the entire seed<br />
surface (about 32%) or on sterile lemmas (about<br />
29%) (Fig. 12).<br />
Microscopic character<br />
a. Mycelium—gray to dark greenish gray, septate.<br />
b. Conidiophores—septate, solitary, or in small<br />
groups; straight or flexuous, sometimes geniculate<br />
(bent like a knee); simple; pale to mid-brown;<br />
bearing conidia at the end and on sides (Fig. 11d).<br />
c. Conidia—dark brown to olivaceous brown,<br />
obclavate, cymbiform, naviculart, fusiform,<br />
straight, or curved (slightly bent on one side). The<br />
largest conidia may have 13 pseudosepta with a<br />
prominent hilum or basal scar (Fig. 11e). Measurements:<br />
5–9 septate, 39.56–101.89 µ × 11.96–<br />
18
Detection frequency (%)<br />
120<br />
100<br />
East Asia<br />
Europe<br />
Latin America<br />
South Asia<br />
Southeast Asia<br />
Sub-Saharan Africa<br />
80<br />
60<br />
40<br />
20<br />
0<br />
Detection level (%)<br />
100<br />
80<br />
60<br />
40<br />
20<br />
0<br />
1990 1991 1992 1993 1994 1995 1996 1997<br />
Year<br />
Fig. 10. Detection frequency (a) and level (b) of Bipolaris oryzae from imported untreated seeds, 1990-97.<br />
16.10 µ (PDA); 4–11 septate, 43.47–101.43 µ ×<br />
12.19–16.10 µ (PSA); and 5–11 septate, 59.80–<br />
106.03 µ × 10.12–16.33 µ (MEA).<br />
Colony characters on culture media (Fig. 13)<br />
Colonies on PDA at ART (28–30 °C) grow slowly<br />
and attain a 3.38-cm diam in 5 d. They are azonated<br />
with sinuate margins, hairy at the center, becoming<br />
cottony toward the margin, yellowish gray at the center<br />
and gray toward the margin, and becoming grayish<br />
olive with age. The colony appears azonated and<br />
black on the reverse side of the agar plate. At 21 °C<br />
under alternating 12-h NUV light and 12-h darkness,<br />
colonies grow very slowly and attain a 2.38-cm diam<br />
in 5 d. They are fluffy, azonated with uneven margins,<br />
with olive gray aerial mycelia, becoming dark<br />
olive gray outward. The colony on the reverse side of<br />
the agar plate appears azonated and black. At 28 °C<br />
under alternating 12-h fluorescent light and 12-h<br />
darkness, colonies grow very slowly and attain a<br />
2.53-cm diam in 5 d. They are fluffy with nil to<br />
scanty aerial mycelia, azonated with uneven margins,<br />
and olive black with 3.0-mm light gray advancing<br />
mycelia. The colony appears azonated and black<br />
with light gray margins on the reverse side of the<br />
agar plate.<br />
Colonies on PSA incubated at ART (28–30 °C)<br />
grow moderately fast and attain a 4.48-cm diam in 5<br />
d. They are fluffy, azonated with sinuate margins,<br />
and grayish yellow at the center, becoming dark olive<br />
gray outward. The colony appears azonated and olive<br />
black to black on the reverse side of the agar<br />
19
→<br />
d<br />
e<br />
a<br />
e<br />
b<br />
d<br />
e<br />
d<br />
d<br />
e→<br />
c<br />
Fig. 11. Habit character of Bipolaris oryzae (Breda de Haan) Shoem. on (a) whole seed (10X), (b) sterile lemmas<br />
(40X), and (c) awn portion (40X). Photomicrograph of B. oryzae showing (d) conidiophore and (e) conidia at 10X and<br />
40X.<br />
Observed frequency (%)<br />
40<br />
30<br />
20<br />
10<br />
0<br />
Sterile<br />
lemmas<br />
Awn<br />
Partition<br />
bet. lemma<br />
and palea<br />
Entire<br />
seed<br />
Lemma/<br />
palea<br />
only or<br />
both<br />
Seed part<br />
Fig. 12. Observed frequency of Bipolaris oryzae<br />
occurrence on the seed.<br />
Fig. 13. Plate cultures of Bipolaris oryzae (Breda de<br />
Haan) Shoem. showing colony growths on PDA, PSA,<br />
and MEA incubated at ART, 21 °C, and 28 °C at 15 d<br />
after inoculation.<br />
plate. At 21 °C under alternating 12-h NUV light and<br />
12-h darkness, colonies spread moderately fast and<br />
attain a 4.62-cm diam in 5 d. They are fluffy, zonated<br />
with sinuate margins, and dark olive gray with olive<br />
gray mycelial tufts and 4-mm grayish advancing<br />
mycelia. The colony appears slightly zonated to zonated,<br />
black, and becomes dark olive gray outward on<br />
the reverse side of the agar plate. At 28 °C under<br />
alternating 12-h fluorescent light and 12-h darkness,<br />
colonies grow fast and attain a 5.10 cm diam in 5 d.<br />
20
They are feathery to slightly fluffy, zonated with<br />
even to slightly uneven margins, and alternating olive<br />
yellow and dark olive with 5-mm light yellow margins.<br />
On the reverse side of the agar plate, the colony<br />
appears azonated to slightly zonated, black, and becomes<br />
dark greenish gray to olive black toward the<br />
margin.<br />
Colonies on MEA at ART (28–30 °C) grow very<br />
slowly and attain a 2.29-cm diam in 5 d. Colonies are<br />
scanty with fluffy aerial mycelia, azonated with uneven<br />
margins, and olive gray with grayish yellow<br />
aerial mycelia. The colony appears azonated and<br />
olive black on the reverse side of the agar plate. At<br />
21 °C under alternating 12-h NUV light and 12-h<br />
darkness, colonies are restricted in growth and attain<br />
a 1.71-cm diam in 5 d. They are azonated with<br />
crenate margins, velvety, and olive black with white<br />
to dark olive mycelial tufts. The colony appears zonated<br />
and olive black to black on the reverse side of<br />
the agar plate. At 28 °C under alternating 12-h fluorescent<br />
light and 12-h darkness, colonies are restricted<br />
in growth and attain a 1.71-cm diam in 5 d.<br />
They are azonated with crenate margins, velvety<br />
with slightly fluffy centers, and dark greenish gray to<br />
olive black. The colony on the reverse side of the<br />
agar plate appears azonated and black.<br />
Cercospora janseana (Racib.) Const.<br />
syn. Cercospora oryzae Miyake<br />
teleomorph: Sphaerulina oryzina Hara<br />
Disease caused: narrow brown leaf spot<br />
a. Symptoms<br />
Short, linear, brown lesions most common on<br />
leaves but also occur on leaf sheaths, pedicels,<br />
and glumes.<br />
b. Occurrence/distribution<br />
The disease has worldwide distribution (Fig. 14).<br />
c. Disease history<br />
The disease was first observed in North America<br />
before 1910 but its detailed description was re-<br />
Fig. 14. Occurrence of narrow brown leaf spot (Ou 1985, Agarwal and Mathur 1988, EPPO 1997).<br />
21
ported in 1910 in Japan. The causal fungus was<br />
named Cercospora oryzae. In 1982, the fungus<br />
was renamed as C. janseana.<br />
d. Importance in crop production<br />
The disease reduces effective leaf area of the<br />
plant and causes premature senescence of infected<br />
leaves and sheaths. Together with leaf<br />
scald, it may cause 0.1% yield loss across all rice<br />
production situations in Asia.<br />
Detection on seed<br />
a. Incubation on blotter<br />
Using the blotter test, C. janseana can be observed<br />
on rice seed 7 d after incubation in NUV<br />
light at 21 °C. The frequency of detection is
Observed frequency (%)<br />
120<br />
100<br />
80<br />
60<br />
40<br />
20<br />
0<br />
Sterile<br />
lemmas<br />
Awn<br />
Partition<br />
bet. lemma<br />
and palea<br />
Entire<br />
se ed<br />
Lemma/<br />
palea<br />
only or<br />
both<br />
Seed part<br />
Fig. 16. Observed frequency of Cercospora janseana<br />
occurrence on the seed.<br />
Fig. 17. Plate cultures of Cercospora janseana (Racib)<br />
Const. showing colony growths of PDA, PJA, and VJA<br />
incubated at ART, 21 °C, and 28 °C at 15 d after<br />
inoculation.<br />
Colony characters on culture media (Fig. 17)<br />
Colonies on PDA at ART (28–30 °C) grow very<br />
slowly and attain a 2.40-cm diam in 17 d. They are<br />
azonated, plane to slightly felted, with sinuate margins,<br />
slightly radial furrows, and dark gray. The<br />
colony appears azonated with radial wrinkles and<br />
black on the reverse side of the agar plate. At 21 °C<br />
under alternating 12-h NUV light and 12-h darkness,<br />
colonies grow very slowly and attain a 2.60-cm diam<br />
in 17 d. They are zonated, plane to felted, with sinuate<br />
margins and radial furrows, and gray and light<br />
gray at the margins. The colony appears azonated<br />
with radial wrinkles and black on the reverse side of<br />
the agar plate. At 28 °C under alternating 12-h fluorescent<br />
light and 12-h darkness, colonies are restricted<br />
in growth and attain a 1.4-cm diam in 17 d.<br />
They are zonated, felted, with even to sinuate margins<br />
and deep radial furrows, and light gray. The<br />
colony appears azonated with wrinkles and black on<br />
the reverse side of the agar plate.<br />
Colonies on prune juice agar (PJA) at ART (28–<br />
30 °C) grow very slowly and attain a 2.40-cm diam in<br />
17 d. They are azonated, plane, powdery to granular<br />
with slightly radial furrows and even margins, and<br />
dark gray to gray and becoming light at the margins.<br />
The colony on the reverse side of the agar plate appears<br />
azonated and black. At 21 °C under alternating<br />
12-h NUV light and 12-h darkness, colonies grow<br />
slowly and attain a 3.10-cm diam in 17 d. They are<br />
slightly zonated, plane, granular, and gray with 0.5-<br />
cm white margins. The colony on the reverse side of<br />
the agar plate appears azonated and black with orange<br />
coloration. At 28 °C under alternating 12-h fluorescent<br />
light and 12-h darkness, colonies grow slowly<br />
and attain a 3.20-cm diam in 17 d. They are plane,<br />
zonated with radial furrows and sinuate margins, and<br />
light gray to gray. The colony on the reverse side of<br />
the agar plate appears azonated with radial wrinkles<br />
and black.<br />
Colonies on V-8 juice agar (VJA) at ART (28–30<br />
°C) are restricted in growth and attain a 2.20-cm<br />
diam in 17 d. They are zonated, felted, with sinuate<br />
margins and deep radial furrows, and light gray to<br />
gray with dark gray margins. The colony on the reverse<br />
side of the agar plate appears azonated with<br />
wrinkles and black. At 21 °C under alternating 12-h<br />
NUV light and 12-h darkness, colonies grow very<br />
slowly and attain a 2.30-cm diam in 17 d. They are<br />
zonated, felted, with even to sinuate margins and<br />
deep radial furrows, and light gray to dark gray. The<br />
colony on the reverse side of the agar plate appears<br />
azonated with wrinkles and black. At 28 °C under<br />
alternating 12-h fluorescent light and 12-h darkness,<br />
colonies grow very slowly and attain a 2.30-cm diam<br />
in 17 d. They are zonated with deep radial furrows<br />
and sinuate margins, felted, and brownish gray. The<br />
colony on the reverse side of the agar plate is<br />
azonated with radial wrinkles and black.<br />
23
Microdochium oryzae (Hashioka & Yokogi) Samuels & Hallett<br />
syn. Gerlachia oryzae (Hashioka & Yokogi) W. Gams.<br />
Rhychosporium oryzae Hashioka & Yokogi<br />
teleomorph: Monographella albescens (Thumen) Parkinson, Sivanesan & C. Booth<br />
syn. Metasphaeria albescens Thum.<br />
Metasphaeria oryzae-sativae Hara<br />
Micronectriella pavgii R.A. Singh<br />
Griposphaerella albescens (Thumen) Von Arx<br />
Disease caused: leaf scald<br />
a. Symptoms<br />
Lesions are usually observed on mature leaves.<br />
Characteristic symptoms include zonated lesions<br />
that start at leaf edges or tips. The lesion shape is<br />
more or less oblong with light brown halos measuring<br />
1–5 cm long and 0.5–1 cm wide. Individual<br />
lesions enlarge and eventually coalesce. As lesions<br />
become old, zonations fade.<br />
b. Occurrence/distribution<br />
Leaf scald has been reported in all rice-growing<br />
countries worldwide (Fig. 18).<br />
c. Disease history<br />
Leaf scald was first reported in 1955 in Japan,<br />
and the causal organism was named as<br />
Rhynchosporium oryzae. However, the disease<br />
was known under different names. The causal<br />
fungus was confused with Fusarium nivale as the<br />
anamorph and with Micronectriella nivalis as the<br />
teleomorph. Later it was proved that the leaf scald<br />
fungus is not F. nivale. The anamorph and<br />
teleomorph of the leaf scald fungus have undergone<br />
many changes and are now known as<br />
Gerlachia oryzae and Monographella albescens,<br />
respectively.<br />
d. Importance in crop production<br />
Leaf scald is very common on rice in tropical<br />
Asia. It is considered a relatively minor problem<br />
causing little yield loss alone in rice production.<br />
Detection on seed<br />
a. Incubation period on blotter<br />
Using the blotter test, M. oryzae can be observed<br />
on rice seeds 7 d after seeding and incubation<br />
under NUV light at 21 °C. The detection frequency<br />
is about 28.2% on seeds coming from<br />
different regions (Fig. 19a,b).<br />
b. Habit character<br />
Aerial mycelia are absent; light pinkish or light<br />
orange to bright orange irregular masses<br />
Fig. 18. Occurrence of leaf scald (Ou 1985, Agarwal and Mathur 1988).<br />
24
Frequency level (%)<br />
120<br />
100<br />
East Asia<br />
Europe<br />
Latin America<br />
South Asia<br />
Southeast Asia<br />
Sub-Saharan Africa<br />
80<br />
60<br />
40<br />
20<br />
0<br />
Detection level (%)<br />
50<br />
40<br />
30<br />
20<br />
10<br />
0<br />
1990 1991 1992 1993 1994 1995 1996 1997<br />
Year<br />
Fig. 19. Detection frequency (a) and level (b) of Microdochium oryzae from imported untreated seeds, 1990-97.<br />
(pionnotes) varying in size and thickness are scattered<br />
on seed surface (Fig. 20a-c).<br />
c. Location on seed<br />
M. oryzae is most likely observed growing on<br />
sterile lemmas of the rice seed (about 55%) (Fig.<br />
21).<br />
Microscopic character<br />
Conidia (epispore)—borne on superficial stromata<br />
arising on lesions, bow-shaped; single-celled when<br />
young, 2-celled when mature; one septum; occasionally<br />
2–3 septate; not considered at septum; thinwalled,<br />
hyaline, pink in mass, hyaline under the microscope<br />
(Fig. 22d). Measurements: 8.97–17.48 µ ×<br />
2.53–5.98 µ (PDA); 8.51–18.17 µ × 6.21–8.51 µ<br />
(PSA); and 10.36–15.64 µ × 2.30–5.52 µ (MEA).<br />
Colony characters on culture media (Fig. 22)<br />
Colonies on PDA at ART (28–30 °C) grow moderately<br />
fast, thinly spreading, and attain a 4.20-cm diam<br />
in 5 d. They are evenly zonated with uneven margins,<br />
orange with scanty, white aerial mycelia, and<br />
somewhat pressed to the media. Colonies appear wet<br />
at the center, spreading outward with age. The<br />
colony on the reverse side of the agar plate appears<br />
evenly zonated and light orange. At 21 °C under alternating<br />
12-h NUV light and 12-h darkness, colonies<br />
are thinly spreading, grow moderately fast, and attain<br />
25
a<br />
b<br />
c<br />
d<br />
Fig. 20. Habit character of Microdochium oryzae (Hashioka and Yokogi) Sam. and Hal. showing orange pionnotes<br />
on the seed surface at (a) 8X, (b) 12.5X, and (c) 20X. cPhotomicrograph of M. oryzae showing lunar-shaped conidia d<br />
(40X).<br />
Observed frequency (%)<br />
60<br />
50<br />
40<br />
30<br />
20<br />
10<br />
0<br />
Sterile<br />
lemmas<br />
Awn<br />
Partition<br />
bet. lemma<br />
and palea<br />
Entire<br />
se ed<br />
Lemma/<br />
palea<br />
only or<br />
both<br />
Seed part<br />
Fig. 21. Observed frequency of Microdochium oryzae<br />
occurrence on the seed.<br />
Fig. 22. Plate cultures of Microdochium oryzae<br />
(Hashioka and Yokogi) Samuels and Hallet showing<br />
colony growths on PDA, PSA, and MEA incubated at<br />
ART, 21 °C, and 28 °C at 5 d after inoculation.<br />
26
a 4.90-cm diam in 5 d. They are evenly zonated,<br />
orange with white aerial mycelia that appear to be<br />
pressed to the media, and wet at the center. The<br />
colony on the reverse side of the agar plate is<br />
slightly zonated and orange to light orange outward.<br />
At 28 °C under alternating 12-h fluorescent light and<br />
12-h darkness, colonies grow moderately fast and<br />
attain a 5.0-cm diam in 5 d. They are orange without<br />
aerial mycelia. Colonies appear wet and slightly<br />
zonated with radial furrows and even margins. The<br />
colony on the reverse side of the agar plate is<br />
slightly zonated with radial wrinkles and orange,<br />
becoming light outward.<br />
Colonies on PSA at ART (28–30 °C) are thinly<br />
spreading, grow moderately fast, and attain a 4.87-<br />
cm diam in 5 d. They are azonated with even margins<br />
and light orange with scarce white aerial mycelia.<br />
White mycelial tufts are produced as colonies<br />
age. The colony on the reverse side of the agar<br />
plate appears azonated and light orange. At 21 °C<br />
under alternating 12-h NUV light and 12-h darkness,<br />
colonies are thinly spreading, grow moderately fast,<br />
and attain a 4.48-cm diam in 5 d. They are slightly<br />
zonated at the center, with even margins, and light<br />
orange with scarce white aerial mycelia that are<br />
pressed to the media. The colony on the reverse<br />
side of the agar plate is slightly zonated at the center<br />
and light orange. At 28 °C under alternating 12-h<br />
fluorescent light and 12-h darkness, colonies grow<br />
moderately fast and attain a 5.89-cm diam in 5 d.<br />
They are zonated at the center with about 1.5-cm<br />
submerged advancing mycelia and sinuate margins.<br />
Colonies are orange with white, densely floccose<br />
aerial mycelia. The colony on the reverse side of the<br />
agar plate appears zonated at the center and orange.<br />
Colonies on MEA at ART (28–30 °C) are thinly<br />
spreading, grow moderately fast, and attain a 4.93-<br />
cm diam in 5 d. They are zonated, with even margins,<br />
and orange with scarce white aerial mycelia<br />
that are somewhat pressed to the media. The colonies<br />
appear wet. The colony on the reverse side of<br />
the agar plate is zonated and orange, At 21 °C under<br />
alternating 12-h NUV light and 12-h darkness, colonies<br />
are thinly spreading, grow moderately fast, and<br />
attain a 5.67-cm diam in 5 d. They are zonated, with<br />
few radial furrows and even margins, and orange<br />
with scarce white aerial mycelia that are somewhat<br />
pressed to the media. The colonies appear wet at the<br />
center and spread outward with age. The colony on<br />
the reverse side of the agar plate appears zonated<br />
with few radial wrinkles and orange. At 28 °C under<br />
alternating 12-h fluorescent light and 12-h darkness,<br />
colonies are thinly spreading, grow fast, and attain a<br />
6.03-cm diam in 5 d. They are zonated with serrated<br />
margins, orange with scarce white aerial mycelia<br />
that are somewhat pressed to the media, especially at<br />
the center, and become wet with age. The colony on<br />
the reverse side of the agar plate appears zonated<br />
with few radial wrinkles and orange.<br />
Pyricularia oryzae Cav.<br />
syn. Pyricularia grisea (Cooke) Sacc.<br />
Pyricularia grisea<br />
Pyricularia oryzae Cavara<br />
Dactylaria oryzae (Cav.) Sawad<br />
Trichothecium griseum Cooke<br />
teleomorph: Magnaporthe grisea (Hebert) Barr<br />
Ceratospaeria grisea Hebert<br />
Phragmoporthe grisea (Hebert) Monod<br />
Disease caused: blast<br />
a. Symptoms<br />
The fungus can infect rice plants at any growth<br />
stage although it is more frequent at the seedling<br />
and flowering stage.<br />
On the leaves—Initially, lesions appear as small<br />
whitish or grayish specks that eventually enlarge<br />
and become spindle-shaped necrotic spots with<br />
brown to reddish brown margins. The size, shape,<br />
and color of the spots vary depending upon the<br />
susceptibility of the variety and environmental<br />
conditions.<br />
On the panicle base—Infected tissue shrivels and<br />
turns black. It breaks easily at the neck and hangs<br />
down.<br />
On the nodes—Infected nodes rot and turn black.<br />
27
. Occurrence/distribution<br />
<strong>Rice</strong> blast is widely distributed in all rice-growing<br />
countries (Fig. 23). It is most prevalent in temperate<br />
subtropical environments and also in rice<br />
grown in upland conditions.<br />
c. Disease history<br />
Records of this disease can be traced back to as<br />
early as 1637 in China. It was reported in 1704 in<br />
Japan, in 1828 in Italy, and in 1907 in South Carolina,<br />
USA. In India, it was first recorded in 1913.<br />
Its causal fungus, Pyricularia oryzae, was named<br />
in 1891 in Italy. It was recently renamed P. grisea<br />
but P. oryzae has widespread usage.<br />
d. Importance in crop production<br />
Blast is generally considered as the principal disease<br />
of rice because of its wide distribution and<br />
destruction in causing crop failure and epidemics.<br />
The epidemic potential is very high under favorable<br />
conditions where susceptible cultivars are<br />
planted. Blast may cause total crop failure but,<br />
because resistant cultivars are grown widely in<br />
major rice production environments, it accounts<br />
for 1–3% yield loss across all rice production situations<br />
in Asia.<br />
Detection on seed<br />
a. Incubation period on blotter<br />
Using the blotter test, P. oryzae can be observed<br />
on rice seeds 3–4 d after incubation in NUV light<br />
at 21 °C. The detection frequency is about 9.9%<br />
on seeds coming from different regions (Fig.<br />
24a,b).<br />
b. Habit character<br />
Aerial mycelia are rarely present or in most cases<br />
absent. If present, mycelia are branched, hyaline<br />
to olivaceous. If aerial mycelium is absent, conidiophores<br />
arise directly from the seed surface singly<br />
or in small groups or bundles. They are moderately<br />
long, simple, and light brown. Conidia are<br />
hyaline, pale olive or grayish, and borne<br />
sympodially (Fig. 25a-c).<br />
c. Location on seed<br />
P. oryzae is observed mostly on sterile lemmas of<br />
the seed (91%) (Fig. 26).<br />
Microscopic characters<br />
a. Mycelium—septate, branched, and hyaline.<br />
b. Conidiophores—simple to rarely branched, moderately<br />
long, septated, light brown, slightly thickened<br />
at the base with denticles at the apex (Fig.<br />
25d).<br />
c. Conidia (sympodulosphores)—pyriform to<br />
obclavate, hyaline to pale olive; usually 2 septate,<br />
rarely 1 or 3 septate (observed in PJA); apex narrow,<br />
base rounded with a prominent appendage or<br />
hilum (Fig. 25e). Measurements: 15.64–22.54 µ ×<br />
7.82–10.81 µ (PDA); 16.56–31.97 µ × 8.51–12.42<br />
µ (PJA); and 15.18–25.76 µ × 7.13–10.81 µ(VJA).<br />
Fig. 23. Occurrence of blast (Ou 1985, CMI 1981).<br />
28
Detection frequency (%)<br />
90<br />
80<br />
East Asia<br />
Europe<br />
Latin America<br />
South Asia<br />
Southeast Asia<br />
Sub-Saharan Africa<br />
70<br />
60<br />
50<br />
40<br />
30<br />
20<br />
10<br />
0<br />
Detection level (%)<br />
35<br />
30<br />
25<br />
20<br />
15<br />
10<br />
5<br />
0<br />
1990 1991 1992 1993 1994 1995 1996 1997<br />
Year<br />
Fig. 24. Detection frequency (a) and level (b) of Pyricularia oryzae from imported untreated seeds, 1990-97.<br />
Colony characters on culture media (Fig. 27)<br />
Colonies on PDA at ART (28–30 °C) grow very<br />
slowly and attain a 3.04-cm diam in 5 d. They are<br />
azonated, slightly felted, with aerial mycelia that are<br />
white with brownish gray portions, even margins, and<br />
with about 1-mm advancing mycelia submerged.<br />
Saltation of colonies is observed in some plates. The<br />
colony on the reverse side of the agar plate is zonated<br />
and black, turning light outward. At 21 °C under<br />
alternating 12-h NUV light and 12-h darkness, colonies<br />
grow very slowly and attain a 2.17-cm diam in 5<br />
d. They are zonated, slightly felted with even margins,<br />
and brownish gray. The colony on the reverse<br />
side of the agar plate appears zonated and black with<br />
a lighter color outward. At 28 °C under alternating<br />
12-h fluorescent light and 12-h darkness, colonies<br />
grow very slowly and attain a 2.78-cm diam in 5 d.<br />
They are azonated and become zonated toward the<br />
margin, floccose to slightly felted. Aerial mycelia are<br />
white with brownish gray portions. The colony on the<br />
reverse side of the agar plate is azonated and becomes<br />
zonated near the margins, and appears white<br />
with greenish gray centers.<br />
Colonies on PJA at ART (28–30 °C) grow very<br />
slowly and attain a 2.87-cm diam in 5 d. They are<br />
azonated, becoming zonated toward the margins,<br />
velvety, becoming granular with age, with 0.8-cm<br />
submerged advancing mycelia, gray to light gray<br />
29
→<br />
a<br />
b<br />
c<br />
d<br />
e<br />
e<br />
→→<br />
e<br />
→<br />
→<br />
Fig. 25. Habit character of Pyricularia oryzae Cav. On sterile lemmas at (a) 10X, (b) 40X, and (c) 50X. Photomicrograph<br />
of P. oryzae showing (d) conidiophore and (e) conidia at 40X.<br />
Observed frequency (%)<br />
100<br />
80<br />
60<br />
40<br />
20<br />
0<br />
Sterile<br />
lemmas<br />
Awn<br />
Partition<br />
bet. lemma<br />
and palea<br />
Seed part<br />
Entire<br />
seed<br />
Lemma/<br />
palea<br />
only or<br />
both<br />
Fig. 26. Observed frequency of Pyricularia oryzae<br />
occurrence on the seed.<br />
Fig. 27. Plate cultures of Pyricularia oryzae showing<br />
colony growths on PDA, PJA, and VJA, incubated at ART,<br />
21 °C, and 28 °C at 15 d after inoculation.<br />
near the margins. The colony on the reverse side of<br />
the agar plate appears azonated and dark purplish<br />
gray. At 21 °C under alternating 12-h NUV light and<br />
12-h darkness, colonies grow very slowly and attain a<br />
2.50-cm diam in 5 d. They are zonated, velvety with<br />
0.5-cm submerged advancing mycelia, and gray,<br />
becoming dark gray outward. The colony on the reverse<br />
side of the agar plate is zonated and dark purplish<br />
gray, becoming lighter outward. At 28 °C under<br />
alternating 12-h fluorescent light and 12-h darkness,<br />
colonies grow very slowly and attain a 3.17-<br />
cm diam in 5 d. They appear slightly zonated and<br />
30
gray, becoming dark near the margins with 1-cm submerged<br />
advancing mycelia. The colony on the reverse<br />
side of the agar plate is slightly zonated and<br />
dark purplish gray, becoming lighter outward.<br />
Colonies on VJA incubated at ART (28–30 °C)<br />
grow very slowly and attain a 2.96-cm diam in 5 d.<br />
They appear azonated, felted with even margins, and<br />
white with light gray portions. The colony on the reverse<br />
side of the agar plate appears azonated and<br />
brown-purple. At 21 °C under alternating 12-h NUV<br />
light and 12-h darkness, colonies grow very slowly<br />
and attain a 2.04-cm diam in 5 d. They appear zonated,<br />
slightly floccose to felted with radial furrows,<br />
and gray, becoming light gray toward the margins.<br />
The colony on the reverse side of the agar plate is<br />
zonated with radial wrinkles and brown-purple,<br />
becoming lighter toward the margin. At 28 °C under<br />
alternating 12-h fluorescent light and 12-h darkness,<br />
colonies grow very slowly and attain a 2.96-cm<br />
diam in 5 d. They appear azonated, becoming<br />
slightly zonated toward the margin, slightly felted<br />
with radial furrows and even margins, and gray,<br />
becoming lighter outward. The colony on the reverse<br />
side of the agar plate is azonated, becoming<br />
zonated toward the margins, with radial wrinkles<br />
and brown-purple, becoming lighter outward.<br />
Seedborne fungi causing stem, leaf sheath, and root diseases in rice<br />
Fusarium moniliforme Sheld.<br />
syn. Fusarium heterosporum Nees<br />
Fusarium verticillioides (Sacc.) Nirenberg<br />
Lisea fujikuroi Sawada<br />
teleomorph: Gibberella fujikuroi (Sawada) S. Ito<br />
Gibberella moniliformis Wineland<br />
Gibberella moniliforme<br />
Disease caused: bakanae, foot rot<br />
a. Symptoms<br />
The most conspicuous and common symptoms<br />
are the bakanae tillers or seedlings—an abnormal<br />
elongation of seedlings that are thin and yellowish<br />
green. These can be observed in the seedbed and<br />
in the field. In mature crops, infected plants may<br />
have a few tall, lanky tillers with pale green flag<br />
leaves; leaves dry up one after the other from<br />
below and eventually die. If the crop survives,<br />
panicles are empty.<br />
b. Occurrence/distribution<br />
The disease is widely distributed in all rice-growing<br />
countries (Fig. 28). The pathogen detected in<br />
Africa is closely associated with that from maize<br />
and sorghum.<br />
c. Disease history<br />
This disease has been known since 1828 in Japan.<br />
In India, the disease was described as causing<br />
foot rot in 1931. Fujikuroi found the teleomorph<br />
and the fungus was placed in the genus<br />
Gibberella as G. fujikuroi with Fusarium<br />
moniliforme as its anamorph.<br />
d. Importance in crop production<br />
The disease can be observed in seedbeds and in<br />
the field. Infected seedlings are either taller than<br />
normal seedlings or stunted. Infected mature<br />
plants eventually wither and die. When such<br />
plants reach the reproductive stage, they bear<br />
empty panicles. Across different rice production<br />
situations, bakanae can cause 0.01% yield loss in<br />
Asia.<br />
Detection on seed<br />
a. Incubation on blotter<br />
Using the blotter test, F. moniliforme can be observed<br />
on rice seeds 5 d after incubating seeds<br />
under NUV light at 21 °C. The detection frequency<br />
is about 28.1% on seeds coming from<br />
different regions (Fig. 29a,b).<br />
b. Habit character<br />
There are abundant aerial mycelia, floccose to<br />
felted, with loose and abundant branching, dirty<br />
white to peach. The conidiophores terminate in<br />
false heads and dirty white to peach pionnotes<br />
may be present (Fig. 30a-c).<br />
31
Fig. 28. Occurrence of bakanae (Ou 1985, Agarwal and Mathur 1988, EPPO 1997).<br />
c. Location on seed<br />
F. moniliforme is most likely observed on the entire<br />
rice seed (about 57%) (Fig. 31).<br />
Microscopic character<br />
a. Mycelia—hyaline, septated (Fig. 30d).<br />
b. Microconidiophore—single, lateral, subulate<br />
phialides formed from aerial hyphae, tapering<br />
toward the apex (Fig. 30e).<br />
c. Macroconidiophore—consisting of a basal cell<br />
bearing 2–3 phialides that produce macroconidia.<br />
d. Microconidia—hyaline, fusiform, ovate or clavate;<br />
slightly flattened at both ends; one- or twocelled;<br />
more or less agglutinated in chains, and<br />
remain joined or cut off in false heads (Fig. 30f).<br />
Measurements: 2.53–16.33 µ × 2.30–5.75 µ<br />
(PDA); 5.06–14.26 µ × 1.61–4.83 µ (PSA); and<br />
4.60–10.35 µ × 1.61–4.83 µ (OA, oatmeal agar).<br />
e. Macroconidia—hyaline, inequilaterally fusoid;<br />
slightly sickle-shaped or almost straight; thinwalled;<br />
narrowed at both ends, occasionally bent<br />
into a hook at the apex and with a distinct foot cell<br />
at the base; 3–5 septate, usually 3 septate, rarely<br />
6–7 septate; formed in salmon orange<br />
sporodochia or pionnotes (Fig. 30g). Measurements:<br />
18.86–40.71 µ × 2.76–4.60 µ (PDA);<br />
16.10–35.42 µ × 2.07–4.60 µ (PSA); and 21.39–<br />
39.56 µ × 2.53–4.60 µ (OA).<br />
Colony characters on culture media (Fig. 32)<br />
Colonies on PDA at ART (28–30 °C) grow moderately<br />
fast and attain a 5.20-cm diam in 5 d. They are<br />
slightly zonated; floccose to slightly felted, and become<br />
powdery with age; white tinged with pink at the<br />
center. The colony appearance on the reverse side of<br />
the agar plate is slightly zonated and white with a purplish<br />
center. At 21 °C under alternating 12-h NUV<br />
light and 12-h darkness, colonies grow slowly and attain<br />
a 3.72-cm diam in 5 d. They are slightly zonated,<br />
cottony to slightly felted with submerged advancing<br />
margins and pink. The colony on the reverse of the<br />
agar plate appears slightly zonated and dark pink and<br />
light toward the margin. At 28 °C under alternating 12-<br />
h fluorescent light and 12-h darkness, colonies grow<br />
moderately fast and attain a 5.10-cm diam in 5 d.<br />
They are zonated and appear cottony to slightly felted<br />
with sinuate margins, purplish at the center and light<br />
outward. Saltation of colonies is occasionally observed<br />
in some plates. The colony on the reverse side<br />
of the agar plate is zonated and purple and light purple<br />
outward.<br />
32
Detection frequency (%)<br />
100<br />
80<br />
East Asia<br />
Europe<br />
Latin America<br />
South Asia<br />
Southeast Asia<br />
Sub-Saharan Africa<br />
60<br />
40<br />
20<br />
0<br />
Detection level (%)<br />
60<br />
50<br />
40<br />
30<br />
20<br />
10<br />
0<br />
1990 1991 1992 1993 1994 1995 1996 1997<br />
Year<br />
Fig. 29. Detection frequency (a) and level (b) of Fusarium moniliforme from imported untreated seeds, 1990-97.<br />
Colonies on PSA at ART (28–30 °C) are spreading<br />
and grow moderately fast, attaining a 5.30-cm<br />
diam in 5 d. They are azonated, floccose with serrate<br />
margins, and white tinged with pink at the center.<br />
The colony on the reverse side of the agar plate is<br />
slightly zonated and white with a purplish tinge at the<br />
center. At 21 °C under alternating 12-h NUV light<br />
and 12-h darkness, colonies grow moderately fast<br />
and attain a 5.34-cm diam in 5 d. They are slightly<br />
zonated, floccose to slightly felted with serrate margins,<br />
and purplish at the center and light purple outward.<br />
The colony on the reverse side of the agar<br />
plate appears slightly zonated and white to creamy.<br />
At 28 °C under alternating 12-h fluorescent light and<br />
12-h darkness, colonies grow moderately fast and<br />
attain a 5.90-cm diam in 5 d. They are slightly zonated,<br />
densely floccose with serrate margins, and<br />
white; they later become creamy at the center. The<br />
colony on the reverse side of the agar plate is slightly<br />
zonated and white to creamy.<br />
Colonies on OA at ART (28–30 °C) grow moderately<br />
fast and attain a 5.78-cm diam in 5 d. They<br />
are azonated and floccose to deeply felted with even<br />
to slightly sinuate margins. Colonies are white and<br />
become purple at the center. The colony on the reverse<br />
side of the agar plate appears azonated and<br />
white with dark purple centers. At 21 °C under alternating<br />
NUV light and 12-h darkness, colonies grow<br />
slowly and attain a 4.93-cm diam in 5 d. They are<br />
zonated, slightly felted with even margins, and white<br />
to purple. Saltation of colonies was observed in some<br />
plates. The colony on the reverse side of the agar<br />
33
a<br />
b<br />
→<br />
d<br />
→<br />
→<br />
→<br />
→<br />
f<br />
→→<br />
e<br />
g<br />
→<br />
→→<br />
→<br />
c<br />
Fig. 30. Habit character of Fusarium moniliforme Sheld. on (a) whole seed (10X) and (b) awn portion (17X). (c)<br />
Mycelial growth of F. moniliforme showing false heads (49X). Photomicrograph of F. moniliforme showing (d)<br />
mycelia, (e) microconidiophores, (f) microconidia, and (g) macroconidia at 40X and stained with lactophenol blue.<br />
→<br />
Observed frequency (%)<br />
120<br />
100<br />
80<br />
60<br />
40<br />
20<br />
0<br />
Sterile<br />
lemmas<br />
Awn<br />
Partition<br />
bet. lemma<br />
and palea<br />
Seed part<br />
Entire<br />
seed<br />
Lemma/<br />
palea<br />
only or<br />
both<br />
Fig. 31. Observed frequency of Fusarium moniliforme<br />
occurrence on the seed.<br />
Fig. 32. Plate cultures of Fusarium moniliforme Sheld.<br />
showing colony growths on PDA, PSA, and oatmeal agar<br />
(OA) incubated at ART, 21 °C, and 28 °C at 15 d after<br />
inoculation.<br />
plate is zonated and white to dark purple. At 28 °C<br />
under alternating 12-h fluorescent light and 12-h<br />
darkness, colonies grow moderately fast and attain a<br />
5.73-cm diam in 5 d. They are slightly zonated, floccose<br />
with even margins, and white with light purplish<br />
coloration at the center. The colony on the reverse<br />
side of the agar plate appears slightly zonated and<br />
dark purple and lighter outward.<br />
34
Sarocladium oryzae (Sawada) W. Gams & D. Hawks.<br />
syn. Acrocylindrium oryzae Saw.<br />
Sarocladium attenuatum W. Gams & D. Hawks.<br />
Disease caused: sheath rot<br />
a. Symptoms<br />
Lesions start at the uppermost leaf sheath enclosing<br />
young panicles as oblong or irregular spots,<br />
with brown margins and gray center or brownish<br />
gray throughout. Spots enlarge and coalesce covering<br />
most of the leaf sheath. Panicles remain<br />
within the sheath or may partially emerge. Affected<br />
leaf sheaths have abundant whitish powdery<br />
mycelium. The pathogen infects rice plants<br />
at all growth stages, but it is most destructive after<br />
the booting stage.<br />
b. Occurrence/distribution<br />
Sarocladium oryzae is present in all rice-growing<br />
countries worldwide (Fig. 33). Sheath rot has become<br />
more prevalent in recent decades and is<br />
very common in rainfed rice or rice during the<br />
rainy season.<br />
c. Disease history<br />
Sawada first described sheath rot of rice in 1922<br />
from Taiwan. He named the causal organism as<br />
Acrocylindrium oryzae. In 1975, Gams and<br />
Hawksworth reclassified the causal organism as<br />
Sarocladium oryzae after comparing their isolates<br />
with those of Sawada.<br />
d. Importance in crop production<br />
Densely planted fields and those infested by stem<br />
borers are susceptible to S. oryzae infection. The<br />
fungus tends to attack leaf sheaths enclosing<br />
young panicles, which retards or aborts the emergence<br />
of panicles. Seeds from infected panicles<br />
become discolored and sterile, thereby reducing<br />
grain yield and quality.<br />
Detection on seed<br />
a. Incubation period on blotter<br />
Using the blotter test, S. oryzae can be observed<br />
on rice seeds 7 d after seeding and incubated under<br />
NUV light conditions at 21 °C. The detection<br />
frequency is about 21.3% on seeds coming from<br />
different regions (Fig. 34a,b).<br />
b. Habit character<br />
The mycelia are white, sparsely branched, septated,<br />
scanty to moderate, creeping close to the<br />
Fig. 33. Occurrence of sheath rot (Ou 1985, EPPO 1997).<br />
35
Detection frequency (%)<br />
120<br />
100<br />
East Asia<br />
Europe<br />
Latin America<br />
South Asia<br />
Southeast Asia<br />
Sub-Saharan Africa<br />
80<br />
60<br />
40<br />
20<br />
0<br />
Detection level (%)<br />
35<br />
30<br />
25<br />
20<br />
15<br />
10<br />
5<br />
0<br />
1990 1991 1992 1993 1994 1995 1996 1997<br />
Year<br />
Fig. 34. Detection frequency (a) and level (b) of Sarocladium oryzae from imported untreated seeds, 1990-97.<br />
seed surface, rarely becoming aerial. Conidiophores<br />
are very short with conidia collected in a<br />
slime drop that are globose and shiny (Fig. 35a-c).<br />
c. Location on seed<br />
S. oryzae is mostly observed on the entire seed<br />
(about 46%) and on the lemma and/or palea<br />
(about 31%) (Fig. 36).<br />
Microscopic character<br />
a. Mycelia—white, sparsely branched, septate (Fig.<br />
35d).<br />
b. Conidiophores—slightly thicker than the vegetative<br />
hyphae, simple, or branched either once or<br />
twice; terminal branches tapering at the tip (Fig.<br />
35e).<br />
c. Conidia—hyaline, smooth, single-celled, cylindrical<br />
with rounded ends; straight, sometimes slightly<br />
curved, formed singly (Fig. 35f). Measurements:<br />
2.07–8.74 µ × 1.15–3.68 µ (PDA); 4.14–8.28 µ ×<br />
1.38–3.68 µ (PSA); and 4.14–7.13 µ ×1.38–3.91 µ<br />
(MEA).<br />
Colony characters on culture media (Fig. 37)<br />
Colonies on PDA at ART (28–30 °C) are restricted in<br />
growth and attain a 4.33-cm diam in 15 d. They are<br />
azonated, plane, velvety with even margins, and pale<br />
36
a<br />
b<br />
c<br />
e<br />
f<br />
d<br />
f<br />
Fig. 35. Habit character of Sarocladium oryzae (Sawada) W. Gams. and D. Hawks. on (a) whole seed (10X), (b) awn<br />
portion (32X), and (c) sterile lemmas (50X) showing minute, shiny, and globose false heads. Photomicrograph of S.<br />
oryzae showing (d) mycelia, (e) conidiophores, and (f) conidia at 40X and stained with lactophenol blue.<br />
Observed frequency (%)<br />
50<br />
40<br />
30<br />
20<br />
10<br />
0<br />
Sterile<br />
lemmas<br />
Awn<br />
Partition<br />
bet. lemma<br />
and palea<br />
Entire<br />
se ed<br />
Lemma/<br />
palea<br />
only or<br />
both<br />
Seed part<br />
Fig. 36. Observed frequency of Sarocladium oryzae<br />
occurrence on the seed.<br />
Fig. 37. Plate cultures of Sarocladium oryzae (Sawada)<br />
W. Gams and D. Hawks. showing colony growths on<br />
PDA, PSA, and MEA incubated at ART, 21 °C, and 28 °C<br />
at 15 d after inoculation.<br />
37
orange. On the reverse side of the agar plate, the<br />
colony looks azonated and yellowish brown. At 21 °C<br />
under alternating 12-h NUV light and 12-h darkness,<br />
colonies are restricted in growth and attain a 3.96-cm<br />
diam in 15 d. They are azonated, plane, velvety with<br />
even to slight sinuate margins, pale orange, and<br />
moisture is produced with age. The colony on the<br />
reverse side of the agar plate appears azonated and<br />
yellowish brown. At 28 °C under alternating 12-h<br />
fluorescent light and 12-h darkness, colonies are restricted<br />
in growth and attain a 4.23-cm diam in 15 d.<br />
They are zonated, plane, velvety with sinuate margins,<br />
and pale orange. On the reverse side of the agar<br />
plate, the colony appears slightly zonated and yellowish<br />
brown.<br />
Colonies on PSA at ART (28–30 °C) are restricted<br />
in growth and attain a 4.80-cm diam in 15 d.<br />
They are slightly zonated, slightly felted with sinuate<br />
margins, and pale orange. The colony on the reverse<br />
side of the agar plate appears slightly zonated and<br />
pale yellow-orange. At 21 °C under alternating 12-h<br />
NUV light and 12-h darkness, colonies are restricted<br />
in growth and attain a 4.21-cm diam in 15 d. They<br />
are azonated, plane, slightly velvety, with a few<br />
slight radial furrows, sinuate margins, and pale orange.<br />
The colony appears azonated, with a few radial<br />
wrinkles and pale yellow-orange on the reverse<br />
side of the agar plate. At 28 °C under alternating 12-h<br />
fluorescent light and 12-h darkness, colonies are restricted<br />
in growth and attain a 4.05-cm diam in 15 d.<br />
They are slightly zonated, slightly felted with a few<br />
slight radial furrows in some plates, with slightly sinuate<br />
to even margins, and pale orange; moisture is<br />
produced with age. The colony appears slightly zonated<br />
with a few slight radial wrinkles and pale yellow-orange<br />
on the reverse side of the agar plate.<br />
Colonies on MEA at ART (28–30 °C) are restricted<br />
in growth and attain a 4.84-cm diam in 15 d.<br />
They are slightly zonated, plane, velvety, and pale<br />
orange. The colony appears slightly zonated and dull<br />
orange with pale yellow-orange margins on the reverse<br />
side of the agar plate. At 21 °C under alternating<br />
12-h NUV light and 12-h darkness, colonies are<br />
restricted in growth and attain a 4.37-cm diam in 15<br />
d. They are zonated, felted with slight sinuate margins,<br />
and pale orange. On the reverse side of the agar<br />
plate, the colony appears azonated and dull orange<br />
with pale yellow-orange margins. At 28 °C under<br />
alternating 12-h fluorescent light and 12-h darkness,<br />
colonies are restricted in growth and attain a 4.47-cm<br />
diam in 15 d. They are plain to felted, zonated at the<br />
center, and become azonated toward the margins,<br />
with slight radial furrows and slight sinuate margins.<br />
Colonies are pale orange and whitish toward the margins.<br />
On the reverse side of the agar plate, the colony<br />
appears zonated with a few radial wrinkles and dull<br />
orange with pale yellow-orange margins.<br />
Seedborne fungi causing grain and inflorescence diseases in rice<br />
Curvularia sp.<br />
Disease caused: black kernel<br />
a. Symptoms<br />
Black discoloration on grains.<br />
b. Occurrence/distribution<br />
Curvularia sp. is frequently isolated from discolored<br />
rice grains. Several species have been reported<br />
on rice from different countries (Fig. 38),<br />
but C. lunata and C. geniculata are the most common<br />
ones.<br />
c. Importance in crop production<br />
Curvularia sp. causes little or no yield loss under<br />
normal rice production situations. Infected grains,<br />
after being polished, may produce black kernels,<br />
thus reducing their market value.<br />
Detection on seed<br />
a. Incubation period on blotter<br />
On blotters incubated under NUV light at 21 °C,<br />
the fungus can be observed growing on rice seed<br />
7 d after seeding. The detection frequency is<br />
about 70.6% on seeds coming from different regions<br />
(Fig. 39a,b).<br />
b. Habit character<br />
Aerial mycelia are scanty or absent; if present,<br />
they are light brown to brown with abundant<br />
branching. Conidiophores are solitary or in groups;<br />
dark brown; straight, sometimes bent; simple;<br />
arising directly from the seed surface. Conidia are<br />
borne more or less at the tip in a whorl or in thick<br />
panicles (Fig. 40a-c).<br />
38
Fig. 38. Occurrence of black kernel (Ou 1985, CABI/EPPO 1997).<br />
c. Location on seed<br />
Curvularia sp. is observed most often on the<br />
lemma and/or palea (about 66%) of the seed (Fig.<br />
41).<br />
Microscopic character<br />
a. Mycelia—septated, branched, subhyaline to light<br />
brown, in some cases dark brown (Fig. 40d).<br />
b. Conidiophores—dark brown, unbranched, septate,<br />
sometimes bent and knotted at the tip (Fig. 40e).<br />
c. Conidia—dark brown, boat-shaped, rounded at the<br />
tip, mostly a little constricted at the base; with<br />
hilum scarcely or not at all protuberant, smoothwalled,<br />
light to dark brown, with three septa; the<br />
2nd cell is larger than the 1st, 3rd, and 4th cells;<br />
bent on the 2nd cell; borne at the tip, arranged in a<br />
whorl one over another or more or less spirally<br />
arranged or in thick panicles (Fig. 40f). Measurements:<br />
16.33–24.84 µ × 7.36–13.34 µ (PDA);<br />
17.48–27.37 µ × 8.28–13.11 µ (PSA); and 15.64–<br />
26.91 µ × 7.36–12.65 µ (MEA).<br />
Colony characters on culture media (Fig. 42)<br />
Colonies on PDA at ART (28–30 °C) grow fast and<br />
attain an 8.40-cm diam in 5 d. Colonies are zonated<br />
and felted; the conidial area is greenish gray with a 3-<br />
mm sterile advancing margin and abundant grayish<br />
mycelial tufts. The colony appearance on the reverse<br />
side of the agar plate is zonated and gray. At 21 °C<br />
under alternating 12-h NUV light and 12-h darkness,<br />
colonies grow moderately fast and attain a 5.94-cm<br />
diam in 5 d. They are cottony to slightly felted with<br />
slight radial furrows and 5-mm even, sterile margins,<br />
zonated, and black, becoming gray toward the margins.<br />
The colony appearance on the reverse side of<br />
the agar plate appears zonated and black at the center<br />
and lighter outward. At 28 °C under alternating<br />
12-h fluorescent light and 12-h darkness, colonies<br />
grow very fast and attain an 8.30-cm diam in 5 d.<br />
Colonies are zonated, hairy to slightly felted, and the<br />
conidial area is olive gray to greenish gray with a 2-<br />
mm sterile white margin. The colony appearance on<br />
the reverse side of the agar plate is slightly zonated<br />
and black.<br />
Colonies on PSA at ART (28–30 °C) grow very<br />
fast and attain an 8.50-cm diam in 5 d. They are<br />
slightly zonated, slightly cottony, and somewhat depressed<br />
to the media. The conidial area is black with<br />
3-mm sterile white margins becoming black as<br />
conidia are produced. The colony on the reverse side<br />
of the agar plate appears zonated and slightly black.<br />
At 21 °C under alternating 12-h NUV light and 12-h<br />
darkness, colonies grow fast and attain a 6.91-cm<br />
diam in 5 d. They are zonated, slightly cottony, with a<br />
39
Detection frequency (%)<br />
120<br />
100<br />
East Asia<br />
Europe<br />
Latin America<br />
South Asia<br />
Southeast Asia<br />
Sub-Saharan Africa<br />
80<br />
60<br />
40<br />
20<br />
0<br />
Detection level (%)<br />
100<br />
80<br />
60<br />
40<br />
20<br />
0<br />
1990 1991 1992 1993 1994 1995 1996 1997<br />
Year<br />
Fig. 39. Detection frequency (a) and level (b) of Curvularia sp. from imported untreated seeds, 1990-97.<br />
black conidial area with 3-mm sterile white margins.<br />
The colony on the reverse side of the agar plate appears<br />
zonated, black, and light outward. At 28 °C<br />
under alternating 12-h fluorescent light and 12-h<br />
darkness, colonies grow very fast and attain a 9.0-cm<br />
diam in 5 d. They are zonated, slightly cottony, and<br />
the conidial area is black with 5-mm sterile white<br />
margins turning black as conidia are produced. The<br />
colony on the reverse side of the agar plate appears<br />
slightly zonated, black, and light outward.<br />
Colonies on MEA at ART (28–30 °C) grow very<br />
fast and attain an 8.17-cm diam in 5 d. They are<br />
markedly zonated, felted, and greenish gray. The<br />
colony on the reverse side of the agar plate appears<br />
zonated and black. At 21 °C under alternating 12-h<br />
NUV light and 12-h darkness, colonies grow moderately<br />
fast and attain a 6.53-cm diam in 5 d. They are<br />
zonated, brown, and light outward. The colony on the<br />
reverse side of the agar plate appears zonated and<br />
brown, becoming lighter outward. At 28 °C under<br />
alternating 12-h fluorescent light and 12-h darkness,<br />
colonies grow very fast and attain an 8.23-cm diam<br />
in 5 d. They are zonated, slightly felted, olivaceous<br />
brown, and become light outward with 2-mm sterile<br />
white margins. The colony on the reverse side of the<br />
agar plate appears slightly zonated and black.<br />
40
a<br />
b<br />
d<br />
→<br />
→<br />
→<br />
e<br />
→<br />
f<br />
→<br />
f<br />
→<br />
d<br />
→<br />
c<br />
Fig. 40. Habit character of Curvularia sp. on (a) whole seed (10X), (b) sterile lemmas (20X), and (c) lemma (32X).<br />
Photomicrograph of Curvularia sp. showing (d) mycelia, (e) conidiophores, and (f) conidia at 40X.<br />
Observed frequency (%)<br />
70<br />
60<br />
50<br />
40<br />
30<br />
20<br />
10<br />
0<br />
Sterile<br />
glumes<br />
Awn<br />
Partition<br />
bet. lemma<br />
and palea<br />
Seed part<br />
Entire<br />
seed<br />
Lemma/<br />
palea<br />
only or<br />
both<br />
Fig. 41. Observed frequency of Curvularia sp. occurrence<br />
on the seed.<br />
Fig. 42. Plate cultures of Curvularia lunata (Wakker)<br />
Boedijin showing colony growths on PDA, PSA, and MEA<br />
incubated at ART, 21 °C, and 28 °C at 15 d after<br />
inoculation.<br />
41
Fusarium solani (Mart.) Sacc.<br />
syn. Fusisporium solani Martius<br />
Fusarium javanicum Koorders<br />
Fusarium solani var. martii (Apel & Wollenw.) Wollenw.<br />
Fusarium solani var. striatum (Sherbakov) Woellenw.<br />
teleomorph: Hyphomyces solani<br />
Nectria haematococca var. brevicona (Wollenw.) Gerlach<br />
Disease caused: none reported in rice<br />
a. Occurrence/distribution<br />
F. solani is a rice seedborne pathogen that occurs<br />
in low frequency. The fungus may be involved in<br />
grain discoloration. However, it is detected on<br />
seed coming from different regions and rice ecosystems.<br />
Detection on seed<br />
a. Incubation on blotter<br />
Using the blotter test, F. solani can be observed<br />
on rice seeds 5 d after incubation in NUV light at<br />
21 °C. The detection frequency is
d<br />
a<br />
b<br />
e<br />
→<br />
→<br />
→<br />
→<br />
→<br />
f<br />
c<br />
g<br />
h<br />
Fig. 43. Habit character of Fusarium solani (Mart.) Sacc. on (a) whole seed (11X) and sterile lemmas at (b) 21X and<br />
(c) 40X showing (d) pionnotes and (e) false heads. Photomicrograph of F. solani showing (f) conidiophore, (g)<br />
macroconidia, and (h) microconidia at 40X stained with lactophenol blue.<br />
Observed frequency (%)<br />
70<br />
60<br />
50<br />
40<br />
30<br />
20<br />
10<br />
0<br />
Sterile<br />
glumes<br />
Awn<br />
Partition<br />
bet. lemma<br />
and palea<br />
Seed part<br />
Entire<br />
seed<br />
Lemma/<br />
palea<br />
only or<br />
both<br />
Fig. 44. Observed frequency of Fusarium solani<br />
occurrence on the seed.<br />
Fig. 45. Plate cultures of Fusarium solani (Mart.) Sacc.<br />
showing colony growths on PDA, PSA, and OA incubated<br />
at ART, 21 °C, and 28 °C at 15 d after inoculation.<br />
43
verse side of the agar plate is zonated. The color is<br />
dark reddish brown. At 21 °C under alternating 12-h<br />
NUV light and 12-h darkness, colonies spread relatively<br />
fast and attain a 5.16-cm diam in 5 d. They are<br />
azonated; aerial mycelia are nil to scanty, slightly<br />
pressed to the media, powdery, becoming creamy<br />
with age, and light yellow at the center, becoming<br />
dull reddish brown n with light gray margins. The<br />
colony on the reverse side of the agar plate appears<br />
azonated and dull reddish brown. At 28 °C under<br />
alternating 12-h fluorescent light and 12-h darkness,<br />
colonies spread relatively fast and attain a 5.28-cm<br />
diam in 5 d. They are zonated with even margins and<br />
aerial mycelia are scanty and hairy, with 6-mm submerged<br />
advancing mycelia. The color is dull brown<br />
to brown, becoming lighter toward the margin. The<br />
colony on the reverse side of the agar plate appears<br />
zonated with a dull reddish brown color.<br />
Nigrospora sp.<br />
teleomorph: Khushia oryzae Huds.<br />
Disease caused: minute leaf and grain spot<br />
a. Symptoms<br />
Presence of numerous minute black pustules<br />
(
Fig. 46. Occurrence of minute leaf and grain spot (EPPO 1997).<br />
Detection frequency (%)<br />
120<br />
100<br />
East Asia<br />
Europe<br />
Latin America<br />
South Asia<br />
Southeast Asia<br />
Sub-Saharan Africa<br />
80<br />
60<br />
40<br />
20<br />
0<br />
Detection level (%)<br />
60<br />
50<br />
40<br />
30<br />
20<br />
10<br />
0<br />
1990 1991 1992 1993 1994 1995 1996 1997<br />
Year<br />
Fig. 47. Detection frequency (a) and level (b) of Nigrospora sp. from imported untreated seeds, 1990-97.<br />
45
a<br />
b<br />
→→<br />
f<br />
→<br />
→<br />
c<br />
e<br />
→<br />
d<br />
→<br />
Fig. 48. Habit character of Nigrospora sp. on (a) whole seed (10X), (b) sterile lemmas (32X), and (c) plea (32X)<br />
showing shiny, black, and globose conidia. Photomicrograph of Nigrosopra sp. showing (d) mycelia, (e) conidiophore,<br />
and (f) conidia at 40X.<br />
Observed frequency (%)<br />
70<br />
60<br />
50<br />
40<br />
30<br />
20<br />
10<br />
0<br />
Sterile<br />
lemmas<br />
Awn<br />
Partition<br />
bet. lemma<br />
and palea<br />
Seed part<br />
Entire<br />
seed<br />
Lemma/<br />
palea<br />
only or<br />
both<br />
Fig. 49. Observed frequency of Nigrospora sp. occurrence<br />
on the seed.<br />
Fig. 50. Plate cultures of Nigrospora sp. showing colony<br />
growths on PDA, PSA, and MEA incubated at ART, 21<br />
°C, and 28 °C at 15 d after inoculation.<br />
46
of the agar plate appears slightly zonated and<br />
black.<br />
Colonies on PSA at ART (28–30 °C) grow<br />
moderately fast and attain a 6.38-cm diam in 5 d.<br />
They are slightly zonated and densely floccose<br />
with sinuate margins, black, and later become light<br />
toward the margins. The colony on the reverse side<br />
of the agar plate appears slightly zonated and<br />
black. At 21 °C under alternating 12-h NUV light<br />
and 12-h darkness, colonies grow fast and attain a<br />
7.78-cm diam in 5 d. They are slightly zonated,<br />
densely floccose, black, and lighter toward the<br />
margins. The colony on the reverse side of the agar<br />
plate appears zonated and black. At 28 °C under<br />
alternating 12-h fluorescent light and 12-h darkness,<br />
colonies grow fast and attain a 7.56-cm diam<br />
in 5 d. They are slightly zonated, densely floccose,<br />
black, and become lighter outward with sinuate<br />
margins. The colony of the reverse side of the agar<br />
plate appears slightly zonated and black.<br />
Colonies on MEA at ART (28–30 °C) grow very<br />
fast and attain an 8.00-cm diam in 5 d. They are zonated,<br />
slightly floccose to felted, grayish to black, and<br />
become lighter outward. The colony on the reverse<br />
side of the agar plate appears zonated and black. At<br />
21 °C under alternating 12-h NUV light and 12-h<br />
darkness, colonies grow moderately fast and attain a<br />
6.53-cm diam in 5 d. They are zonated, slightly<br />
felted, and alternating white and light gray. The<br />
colony of the reverse side of the agar plate appears<br />
zonated, dark gray, and light toward the margins. At<br />
28 °C under alternating 12-h fluorescent light and 12-<br />
h darkness, colonies spread fast and attain a 9.00-cm<br />
diam in 5 d. They are zonated, felted, and alternating<br />
gray and light gray. The colony on the reverse side of<br />
the agar plate appears zonated and dark gray.<br />
Phoma sorghina (Sacc.) Boerema et al<br />
teleomorph: Mycosphaerella holci Tehon<br />
Disease caused: glume blight<br />
a. Symptoms<br />
Lesions are initially small, oblong, and brown,<br />
then gradually enlarge and coalesce, becoming<br />
whitish with small black dots.<br />
The fungus infects glumes during the second or<br />
third week following emergence of panicles.<br />
When infection occurs early, no grain is formed.<br />
On the other hand, when infection is late, grains<br />
are partially filled or become discolored and<br />
brittle.<br />
b. Occurrence/distribution<br />
This is a disease of the grain. It is widely distributed<br />
and the pathogen is often detected on rice<br />
seed from different regions and rice production<br />
ecosystems (Fig. 51).<br />
c. Disease history<br />
The disease was first reported in the U.S. and<br />
Japan and later reported in other rice-growing<br />
areas as well. The fungus P. sorghina has been<br />
reported under different names, including<br />
Phyllosticta glumarum (Ell. & Tracy) Miyake,<br />
Ph. oryzina Padw., and Ph. glumicola (Speg.)<br />
Hara, and Phoma oryzicola Hara with<br />
Trematosphaerella oryzae (Miyake) Padw. as its<br />
teleomorph.<br />
d. Importance in crop production<br />
The disease is a relatively minor problem of rice.<br />
Together with other diseases of the grain, the loss<br />
is
Fig. 51. Occurrence of glume blight (EPPO 1997).<br />
b. Pycnidia—dark brown, globose or subglobose<br />
with protruding ostioles (Fig. 53d).<br />
c. Conidia—oblong to ovoid, hyaline to slightly pigmented,<br />
single-celled (Fig. 53e). Measurements:<br />
2.99–6.21 µ × 1.84–3.68 µ (PDA); 3.68–8.74 µ ×<br />
1.84–7.59 µ (PSA); and 3.45–6.67 µ × 1.38–4.60 µ<br />
(MEA).<br />
Colony characters on culture media (Fig. 55)<br />
Colonies on PDA at ART (28–30 °C) spread very<br />
fast and attain a 7.03-cm diam in 5 d. They are<br />
slightly zonated with even margins, thickly felted,<br />
and brownish gray. The colony on the reverse side of<br />
the agar plate appears zonated and is brownish gray<br />
with brownish black spots. At 21 °C under alternating<br />
12-h NUV light and 12-h darkness, colonies spread<br />
very fast and attain a 7.73-cm diam in 5 d. They are<br />
zonated with even margins, felted, dull yellowish<br />
brown at the center, and greenish gray outward with<br />
4-mm light brownish gray advancing margins. The<br />
colony on the reverse side of the agar plate appears<br />
zonated and dark reddish brown at the center and<br />
reddish orange outward. At 28 °C under alternating<br />
12-h fluorescent light and 12-h darkness, colonies<br />
grow very fast and attain an 8.11-cm diam in 5 d.<br />
They are zonated, cottony to felted with even margins,<br />
and grayish olive and light gray outward. On the<br />
reverse side of the agar plate, the colony appears<br />
zonated and alternating brownish black and dull yellow-orange.<br />
Colonies on PSA at ART (28–30 °C) spread<br />
very fast and attain a 7.52-cm diam in 5 d. They are<br />
azonated and fluffy to slightly floccose with even<br />
margins. The color is grayish yellow-brown at the<br />
center, becoming dark grayish yellow to grayish yellow.<br />
On the reverse side of the agar plate, the colony<br />
appears slightly zonated to zonated and is dull yellowish<br />
brown to brownish black with dull yelloworange<br />
margins. At 21 °C under alternating 12-h<br />
NUV light and 12-h darkness, colonies spread very<br />
fast and attain a 7.58-cm diam in 5 d. They are<br />
azonated to slightly zonated, felted to cottony with<br />
even margins, and grayish yellow and gray outward.<br />
On the reverse side of the agar plate, the colony appears<br />
zonated, black at the center, and alternating<br />
dark olive and grayish olive outward. At 28 °C under<br />
alternating 12-h fluorescent light and 12-h darkness,<br />
colonies spread very fast and attain a 7.70-cm diam<br />
in 5 d. They are azonated with even margins, cottony<br />
to fluffy, and olive black, becoming light gray outward.<br />
On the reverse side of the agar plate, colony<br />
appears zonated. The color is black, becoming<br />
brownish black to dull yellow brown toward the margins.<br />
Colonies on MEA at ART (28–30 °C) spread<br />
very fast and attain a 6.68-cm diam in 5 d. They are<br />
48
Detection frequency (%)<br />
120<br />
100<br />
East Asia<br />
Europe<br />
Latin America<br />
South Asia<br />
Southeast Asia<br />
Sub-Saharan Africa<br />
80<br />
60<br />
40<br />
20<br />
0<br />
Detection level (%)<br />
70<br />
60<br />
50<br />
40<br />
30<br />
20<br />
10<br />
0<br />
1990 1991 1992 1993 1994 1995 1996 1997<br />
Year<br />
Fig. 52. Detection frequency (a) and level (b) of Phoma sp. from imported untreated seeds, 1990-97.<br />
azonated and loosely floccose to hairy with even<br />
margins. Aerial mycelia are pressed to the media,<br />
olive black at the center, and become grayish olive to<br />
olive yellow outward. On the reverse side of the agar<br />
plate, the colony appears zonated. It is dark olive at<br />
the center and becomes grayish olive to olive yellow<br />
toward the margins. At 21 °C under alternating 12-h<br />
NUV light and 12-h darkness, colonies are thin but<br />
spread very fast and attain a 6.89-cm diam in 5 d.<br />
They are azonated with even margins. Aerial mycelia<br />
are pressed to the media. The color is dark olive<br />
green at the center and grayish olive outward. On the<br />
reverse side of the agar plate, the colony appears<br />
azonated. The color is olive black at the center and<br />
dark olive outward. At 28 °C under alternating 12-h<br />
fluorescent light and 12-h darkness, colonies spread<br />
thinly but very fast and attain a 7.10-cm diam in 5 d.<br />
They are azonated to slightly zonated, hairy to<br />
loosely floccose with even submerged margins, and<br />
grayish olive. On the reverse side of the agar plate,<br />
the colony appears slightly zonated and is dark olive,<br />
becoming lighter outward.<br />
49
a<br />
b<br />
e<br />
c<br />
e<br />
→<br />
d<br />
Fig. 53. Habit character of Phoma sorghina (Sacc.) on (a) whole seed (10X), (b) palea and lemma (25X), and (c)<br />
sterile lemmas (40X) showing dark, globose to subglobose, ostiolate pycnidia. Photomicrograph of P. sorghina<br />
showing (d) pycnidia and (e) conidia at 40X.<br />
Observed frequency (%)<br />
40<br />
30<br />
20<br />
10<br />
0<br />
Sterile<br />
lemmas<br />
Awn<br />
Partition<br />
bet. lemma<br />
and palea<br />
Seed part<br />
Entire<br />
seed<br />
Lemma/<br />
palea<br />
only or<br />
both<br />
Fig. 54. Observed frequency of Phoma sp. occurrence<br />
on the seed.<br />
Fig. 55. Plate cultures of Phoma sp. showing colony<br />
growths on PDA, PSA, and MEA incubated at ART, 21<br />
°C, and 28 °C at 15 d after inoculation.<br />
50
Pinatubo oryzae Manandhar & Mew<br />
Disease caused: seed rot<br />
a. Symptoms<br />
Gray lesions on plumules.<br />
b. Occurrence/distribution<br />
Pinatubo oryzae is frequently encountered in rice<br />
seed grown in the Philippines and other countries<br />
occurring on both germinated and nongerminating<br />
seeds (Fig. 56).<br />
c. Disease history<br />
This fungus was previously identified as Verticillium<br />
cinnabarinum and re-identified as Pinatubo<br />
oryzae in 1996. It has been detected from rice<br />
seeds since 1982. It is highly probable that the<br />
organism was already present earlier but there are<br />
no literatures to document any efforts to identify<br />
the fungus.<br />
d. Importance in crop production<br />
This fungus is a rice grain pathogen. It is minor in<br />
importance to rice production.<br />
→<br />
Detection on seed<br />
a. Incubation period on blotter<br />
Using the blotter test, P. oryzae can be observed<br />
on rice seeds 5 d after incubation in NUV light at<br />
21 °C. The detection frequency is about 25.2% on<br />
rice seeds coming from different regions.<br />
b. Habit character<br />
Aerial mycelia are sparse to abundant and white<br />
with loose and abundant branching. Conidia are<br />
borne terminally and arranged in a flower-like<br />
manner. Pionnotes present on the seed surface<br />
are wet and creamy to pink or they hang under a<br />
thin cover of aerial hyphae (Fig. 57 a-c).<br />
c. Location on seed<br />
P. oryzae is most often observed over the entire<br />
seed surface (about 46%) (Fig. 58).<br />
Microscopic character<br />
a. Mycelia—hyaline, septate (Fig. 57d).<br />
b. Conidiophore—simple or branched, short, septate<br />
with denticles at the terminal portion (Fig. 57e).<br />
c. Conidia—elongately oval, single- to 2-celled,<br />
very rarely 3-celled; pointed at the basal portion<br />
and rounded at the apical portion, hyaline (Fig.<br />
57f). Measurements: 5.06–10.81 µ × 2.70–6.21 µ<br />
(PDA); 5.75–12.88 µ × 2.76–5.98 µ (PSA); and<br />
5.75–11.73 µ × 2.53–5.06 µ (MEA).<br />
Colony characters on culture media (Fig. 59)<br />
Colonies on PDA at ART (28–30 °C) grow relatively<br />
fast and attain a 5.02-cm diam in 5 d. They are zonated<br />
with even margins, floccose, and reddish or-<br />
Fig. 56. Occurrence of Pinatubo oryzae on rice seed from different countries received at IRRI (IRRI-SHU unpublished<br />
data 1990-97).<br />
51
a<br />
b<br />
→<br />
→<br />
→<br />
f<br />
e<br />
f<br />
c<br />
d<br />
Fig. 57. Habit character of Pinatubo oryzae Manandhar and Mew on (a) whole seed (12X), (b) sterile lemmas (50X),<br />
and (c) awn portion (50X). Photomicrograph of P. oryzae showing (d) mycelia, (e) conidiophore, and (f) conidia at<br />
40X and stained with lactophenol blue.<br />
Observed frequency (%)<br />
60<br />
50<br />
40<br />
30<br />
20<br />
10<br />
0<br />
Sterile<br />
lemmas<br />
Awn<br />
Partition<br />
bet. lemma<br />
and palea<br />
Entire<br />
seed<br />
Lemma/<br />
palea<br />
only or<br />
both<br />
Seed part<br />
Fig. 58. Observed frequency of Pinatubo oryzae<br />
occurrence on the seed.<br />
Fig. 59. Plate cultures of Pinatubo oryzae Manandhar<br />
and Mew showing colony growths on PDA, PSA, and<br />
MEA incubated at ART, 21 °C, and 28 °C at 15 d after<br />
inoculation.<br />
52
ange with orange. The pionnotes are wet. On the<br />
reverse side of the agar plate, the colony appears<br />
slightly zonated and becomes azonated toward the<br />
margins. The color is orange to light yellow-orange<br />
toward the margins. At 21 °C under alternating 12-h<br />
NUV light and 12-h darkness, colonies grow fast and<br />
attain a 6.26-cm diam in 5 d. They are azonated with<br />
even margins and pale orange to grayish red.<br />
Pionnotes are wet and appear as reddish orange<br />
small dots. The colony appears azonated to slightly<br />
zonated on the reverse side of the agar plate. The<br />
color is orange interspersed with dull reddish brown.<br />
At 28 °C under alternating 12-h fluorescent light and<br />
12-h darkness, colonies grow relatively fast and attain<br />
a 5.20-cm diam in 5 d. They are zonated with<br />
even margins, floccose, and alternating pale orange<br />
and orange with pale orange mycelial tufts. The<br />
colony appears slightly zonated to zonated and is<br />
alternating orange and light yellow in color on the<br />
reverse side of the agar plate.<br />
Colonies on PSA at ART (28–30 °C) grow relatively<br />
fast and attain a 5.40-cm diam in 5 d. They are<br />
slightly zonated with even margins, slightly felted,<br />
and orange to light yellow-orange, becoming reddish<br />
brown with age. The colony appears slightly zonated<br />
on the reverse side of the agar plate. The color is<br />
orange to bright reddish brown, becoming light yellow-orange<br />
toward the margins. At 21 °C under alternating<br />
12-h NUV light and 12-h darkness, colonies<br />
grow relatively fast and attain a 5.70-cm diam in 5 d.<br />
They are azonated with even margins and slight radial<br />
furrows, felted, and pale orange with shiny reddish<br />
orange pionnotes. The colony appears<br />
azonated to slightly zonated and alternating yelloworange<br />
and orange on the reverse side of the agar<br />
plate. At 28 °C under alternating 12-h fluorescent<br />
light and 12-h darkness, colonies grow relatively<br />
fast and attain a 5.33-cm diam in 5 d. They are<br />
azonated to slightly zonated with even margins,<br />
slightly felted to fluffy, becoming wet with age, and<br />
pale orange to orange. The colony appears slightly<br />
zonated and orange on the reverse side of the agar<br />
plate.<br />
Colonies on MEA at ART (28–30 °C) grow<br />
moderately fast and attain a 4.92-cm diam in 5 d.<br />
They are azonated with even margins, floccose,<br />
and light yellow-orange, becoming powdery with<br />
age. On the reverse side of the agar plate, the<br />
colony appears slightly zonated and pale yellow to<br />
yellow. At 21 °C under alternating 12-h NUV light<br />
and 12-h darkness, colonies grow relatively fast and<br />
attain a 5.18-cm diam in 5 d. They are azonated<br />
with even margins and thin aerial mycelia that are<br />
pressed to the media. The color is pale orange. The<br />
colony appears azonated and dull yellow-orange on<br />
the reverse side of the agar plate. At 28 °C under<br />
alternating 12-h fluorescent light and 12-h darkness,<br />
colonies grow moderately fast and attain a 4.77-cm<br />
diam in 5 d. They are zonated with even margins.<br />
Aerial mycelia are thin and pressed to the media.<br />
The color is pale orange and becomes powdery<br />
with age. On the reverse side of the agar plate, the<br />
colony appears slightly zonated to zonated and the<br />
color is pale orange.<br />
Tilletia barclayana (Bref.) Sacc. & Syd.<br />
syn. Neovossia barclayana Bref.<br />
Tilletia horrida Tak.<br />
Neovossia horrida (Tak.) Padw. & Kahn<br />
Disease caused: kernel smut (bunt)<br />
a. Symptoms<br />
Infected grains show very small black pustules or<br />
streaks bursting through the glumes. When infection<br />
is severe, rupturing glumes produce a short<br />
beak-like outgrowth or the entire grain is replaced<br />
by powdery black mass of smut spores.<br />
b. Occurrence/distribution<br />
The disease is known to occur in many countries<br />
worldwide (Fig. 60).<br />
c. Disease history<br />
In 1986, the causal fungus of this disease was<br />
originally called Tilletia horrida. Later it was<br />
identified as Neovossia barclayana. Further studies<br />
made placed it in the genus Tilletia; it is now<br />
known as Tilletia barclayana.<br />
d. Importance in crop production<br />
The disease can be observed in the field at the<br />
mature stage of the rice plant. It is considered<br />
economically unimportant, causing stunting of<br />
53
seedlings and reduction in tillers and yield when<br />
smutted seeds are planted.<br />
Detection on seed<br />
a. Dry seed inspection<br />
Infection on seeds can be detected by direct inspection<br />
using a stereo binocular microscope (Fig.<br />
61a,b).<br />
b. Habit character<br />
Aerial mycelia absent. Dull black and globose<br />
teliospores scattered on seed surface and cotyledon<br />
(Fig. 62a-c).<br />
c. Microscopic character<br />
Teliospores are globose to subglobose, light to<br />
dark brown with spines, and measure 22.5–26.0 µ<br />
× 18.0–22.0 µ (Fig. 62d).<br />
Fig. 60. Occurrence of kernel smut (Ou 1985, CMI 1991).<br />
54
Detection frequency (%)<br />
70<br />
60<br />
East Asia<br />
Europe<br />
Latin America<br />
South Asia<br />
Southeast Asia<br />
Sub-Saharan Africa<br />
50<br />
40<br />
30<br />
20<br />
10<br />
0<br />
Detection level (%)<br />
100<br />
80<br />
60<br />
40<br />
20<br />
0<br />
1990 1991 1992 1993 1994 1995 1996 1997<br />
Year<br />
Fig. 61. Detection frequency (a) and level (b) of Tilletia barclayana from imported untreated seeds, 1990-97.<br />
55
a<br />
b<br />
c<br />
d<br />
Fig. 62. Habit character of Tilletia barclayana (Bref.) Sacc. and Syd. (Duran and Fischer) on (a) whole seed (16X),<br />
(b) palea (40X), and (c) cotyledon and portion of lemma (40X). Photomicrograph of T. barclayana showing (d)<br />
teliospores (40X).<br />
56
Other fungi detected on rice seeds<br />
Other fungi are detected on rice seeds from different countries. Some, such as Nakataea sigmoidea, the<br />
conidial state of Sclerotium rolfsii, cause stem rot, which is important in specific ecosystems. However, most<br />
of these “other fungi” are not known to cause diseases of economic importance. These fungi are listed in<br />
Table 5 and photomicrographs of their habit and microscopic characters are shown.<br />
Table 5. List of other fungi detected on rice seeds.<br />
Fungi Incidence a<br />
Acremoniella atra +<br />
Acremoniella verrucosa +<br />
Alternaria longissima ++<br />
A. tenuissima +<br />
Aspergillus clavatus +<br />
A. flavus-oryzae ++<br />
A. niger ++<br />
Chaetomium globosum +<br />
Cladosporium sp. ++<br />
Curvularia eragrostidis +<br />
Drechslera hawaiiensis +<br />
Epicoccum purpurascens +<br />
Fusarium avenaceum +<br />
F. equiseti +<br />
F. larvarum +<br />
F. nivale +<br />
F. semitectum +++<br />
Gilmaniella humicola +<br />
Memnoniella sp. +<br />
Microascus cirrosus +<br />
Monodictys putredinis +<br />
Myrothecium sp. +<br />
Nakataea sigmoidea ++<br />
Nectria heamatococca +<br />
Papularia sphaerosperma +<br />
Penicillium sp. ++<br />
Pestalotia sp. +<br />
Phaeoseptoria sp. +<br />
Phaeotrichoconis crotolariae +<br />
Pithomyces sp. ++<br />
Pyrenochaeta sp. +<br />
Rhizopus sp. ++<br />
Septogloeum sp. +<br />
Sordaria fimicola +<br />
Spinulospora pucciniiphila +<br />
Sterigmatobotrys macrocarpa +<br />
Taeniolina sp. +<br />
Tetraploa aristata +<br />
Trichoderma sp. +<br />
Trichothecium sp. +<br />
Tritirachium sp. +<br />
Ulocladium botrytis +<br />
a<br />
+ = low, ++ = moderate, +++ = frequent.<br />
57
a<br />
b<br />
e<br />
e<br />
d<br />
e<br />
f<br />
c<br />
f<br />
Fig. 63. Habit character of Acremoniella atra (Corda) Sacc. on (a) whole seed (10X) and palea at (b) 25X and (c) 40X.<br />
Photomicrograph of A. atra showing (d) mycelia, (e) conidiophores, and (f) conidia at 10X and stained with<br />
lactophenol blue.<br />
a<br />
b<br />
d<br />
→<br />
→<br />
→<br />
e<br />
c<br />
d<br />
Fig. 64. Habit character of Acremoniella verrucosa Tognini on (a) whole seed (12X) and awn area at (b) 25X and (c)<br />
50X. Photomicrograph of A. verrucosa showing (d) conidiophores and (e) conidia at 40X.<br />
58
a<br />
b<br />
e<br />
c<br />
d<br />
Fig. 65. Habit character of Alternaria longissima Deighton & MacGarvie on (a) whole seed (10X), (b) lemma (40X),<br />
and (c) awn (40X). Photomicrograph of A. longissima showing (d) conidiophore and (e) conidia at 40X.<br />
a<br />
b<br />
c<br />
d<br />
Fig. 66. Habit character of Alternaria tenuissima (Kunze ex Pers.) Wiltshire on awn area at (a) 9X, (b) 25X, and (c)<br />
50X. Photomicrograph of A. tenuissima showing (d) conidia (40X).<br />
59
a<br />
b<br />
→<br />
→<br />
e<br />
c<br />
d<br />
Fig. 67. Habit character of Aspergillus clavatus Desmazieres on palea and lemma at (a) 10X, (b) 25X, and (c) 40X.<br />
Photomicrograph of A. clavatus showing (d) conidiophore and (e) conidial head at 40X and stained with lactophenol<br />
blue.<br />
a<br />
b<br />
f<br />
c<br />
d<br />
e<br />
Fig. 68. Habit character of Aspergillus flavus-oryzae Thom & Raper on (a) whole seed (8X) and lemma at (b) 16X and<br />
(c) 30X. Photomicrograph of A. flavus-oryzae showing (d) conidiophore, (e) conidial head showing sterigmata, and<br />
(f) conidia at 40X.<br />
60
a<br />
d<br />
d<br />
b<br />
c<br />
Fig. 69. Habit character of Aspergillus niger van Tiegh. showing black conidial heads on whole seed at (a) 9X and<br />
(b) 25X. Photomicrograph of A. niger showing (c) portion of conidiophore and (d) conidial head showing sterigmata<br />
and conidia at 40X.<br />
a<br />
b<br />
d<br />
c<br />
Fig. 70. Habit character of Chaetomium globosus Kunze. Fr. showing dark, ostiolate, sub-globose perithecium<br />
with brown flexuous hairs at (a) awn area (40X) and (b) sterile lemma (50X). Photomicrograph of C. globosum<br />
showing (c) perithecium with hairs (40X) and (d) mature ascospores (10X).<br />
61
→<br />
→<br />
→<br />
→<br />
a<br />
b<br />
→<br />
d<br />
→<br />
→<br />
e<br />
→<br />
a<br />
Fig. 71. Habit character of Cladosporium sp. on (a) embryonal area (10X) and sterile lemmas at (b) 40X and (c) 50X.<br />
Photomicrograph of Cladosporium sp. showing portion of (d) conidiophores and (e) conidia at 40X.<br />
a<br />
b<br />
d<br />
d<br />
d<br />
→<br />
→<br />
e<br />
e<br />
→<br />
c<br />
Fig. 72. Habit character of Curvularia eragrostidis (P. Henn.) Meyer on (a) whole seed (9X) and lemma at (b) 25X and<br />
(c) 50X. Photomicrograph of C. eragrostidis showing (d) conidiophore and (e) conidia at 40X.<br />
62
→<br />
→<br />
→<br />
a<br />
b<br />
f<br />
f<br />
e<br />
d<br />
e<br />
e<br />
c<br />
f<br />
Fig. 73. Habit character of Drechslera hawaiiensis Subram. & Jain on (a) whole seed (9X) and lemma at (b) 25X and<br />
(c) 50X. Photomicrograph of D. hawaiiensis showing (d) mycelia, (e) conidiophores, and (f) conidia at 40X.<br />
a<br />
→<br />
b<br />
d<br />
→<br />
→<br />
c<br />
Fig. 74. Habit character of Epicoccum purpurascens Ehrenb. ex Schlect. on sterile lemmas showing sporodochia<br />
at (a) 10X, (b) 25X, and (c) 50X. Photomicrograph of E. purpurascens showing (d) golden brown conidia (40X).<br />
63
a<br />
b<br />
c<br />
Fig. 75. Habit character of Fusarium avenaceum (Corda ex Fr.) Sacc. on whole seed at (a) 12X and (b) 40X showing<br />
white floccose aerial mycelia with pionnotal-like sporodochia. Photomicrograph of F. avenaceum showing (c)<br />
conidia (40X) stained with lactophenol blue.<br />
64
a<br />
b<br />
a<br />
Fig. 76. Habit character of Fusarium equiseti (Corda) Sacc. showing light orange pionnotes on (a) whole seed (10X)<br />
and (b) sterile lemmas and palea and lemma (25X). Photomicrograph of F. equiseti showing (c) falcate conidia<br />
(40X) stained with lactophenol blue.<br />
65
a<br />
→<br />
→<br />
→<br />
→<br />
→<br />
→<br />
a<br />
f<br />
→<br />
d<br />
b<br />
→<br />
f<br />
c<br />
e<br />
→<br />
Fig. 77. Habit character of Fusarium larvarum Fuckel on embryonal area showing slimy yellowish pionnote at (a)<br />
10X, (b) 18X, and (c) 35X. Photomicrograph of F. larvarum showing (d) mycelia, (e) conidiophore, and (f) conidia<br />
(40X) stained with lactophenol blue.<br />
→<br />
→<br />
a<br />
b<br />
c<br />
d<br />
Fig. 78. Habit character of Fusarium nivale Ces. showing sporodochia on embryonal area at (a) 12X, (b) 25X, and<br />
(c) 40X. Photomicrograph of F. nivale showing (d) conidia (40X) stained with lactophenol blue.<br />
66
a<br />
b<br />
d<br />
c<br />
d<br />
e<br />
e<br />
Fig. 79. Habit character of Fusarium semitectum Berk. & Rav. on (a) whole seed (10X), (b) awn portion (25X), and<br />
(c) lemma (50X). Photomicrograph of F. semitectum showing (d) conidiophores and (e) macroconidia at 40X and<br />
stained with lactophenol blue.<br />
a<br />
b<br />
d<br />
c<br />
d<br />
Fig. 80. Habit character of Gilmaniella humicola Barron on sterile lemmas at (a) 9X, (b) 25X, and (c) 50X.<br />
Photomicrograph of G. humicola showing (d) conidia at 40X.<br />
67
→<br />
a<br />
b<br />
f<br />
→<br />
→<br />
→<br />
f<br />
→<br />
e<br />
→<br />
→<br />
e<br />
d<br />
c<br />
→<br />
d<br />
Fig. 81. Habit character of Memmoniella sp. on sterile lemmas at (a) 10X, (b) 25X, and (c) 40X. Photomicrograph<br />
of Memmoniella sp. showing (d) conidiophores, (e) phialides, and (f) conidia at 40X.<br />
a<br />
b<br />
e<br />
c<br />
d<br />
Fig. 82. Habit character of Microascus cirrosus showing dark, globose, ostiolate, with cylindrical neck ascoma on<br />
(a) whole seed (8X) and lemma and sterile lemmas at (b) 19X and (c) 40X. Photomicrograph of M. cirrosus showing<br />
(d) portion of ascoma and (e) mature ascopores at 40X.<br />
68
a<br />
b<br />
c<br />
→<br />
→<br />
→<br />
d →<br />
Fig. 83. Habit character of Monodictys putredinis (Wallr.) Hughes showing blackish brown aerial mycelia and<br />
almost black conidia on whole seed at (a) 10X and (b) 50X. Photomicrograph of M. putredinis showing (c)<br />
conidiophore and (d) conidia at 40X.<br />
69
→<br />
→<br />
→<br />
→<br />
→<br />
→<br />
→<br />
→<br />
→<br />
→<br />
→<br />
→<br />
a<br />
b<br />
→<br />
c<br />
d<br />
Fig. 84. Habit character of Myrothecium sp. on palea and lemma at (a) 10X, (b) 25X, and (c) 50X showing cushionlike<br />
sporodochia with marginal hyaline setae. Photomicrograph of Myrothecium sp. showing (d) elongately ovoid<br />
conidia (40X) stained with lactophenol blue.<br />
a<br />
d<br />
b<br />
c<br />
Fig. 85. Habit character of Nakataea sigmoidea Hara on sterile lemmas and pedicel at (a) 8X and (b) 50X.<br />
Photomicrograph of N. sigmoidea showing (c) conidiophore and (d) conidia at 40X.<br />
70
→<br />
→<br />
→<br />
a<br />
b<br />
d<br />
c<br />
Fig. 86. Habit character of Nectria haematococca Berk. & Broome showing superficial, red-orange, globose<br />
ascoma at (a) 20X and (b) 40X. Photomicrograph of N. haematococca showing (c) cross section of ascoma (10X)<br />
and (d) ascopores (40X) stained with lactophenol blue.<br />
a<br />
b<br />
d<br />
c<br />
Fig. 87. Habit character of Papularia sphaerosperma (Pers.) Hohnel. showing minute, black, round conidia at (a)<br />
8X, (b) 25X, and (c) 50X. Photomicrograph of P. sphaerosperma showing (d) conidia (63X).<br />
71
a<br />
b<br />
f<br />
e<br />
c<br />
d<br />
Fig. 88. Habit character of Penicillium sp. on (a) whole seed (10X), (b) sterile lemmas and lemma (18X), and (c) awn<br />
(50X). Photomicrograph of Penicillium sp. showing (d) branched conidiophore, (e) phialides, and (f) conidia at OIO.<br />
72
a<br />
b<br />
c<br />
Fig. 89. Habit character of Pestalotia sp. showing subepidermal acervuli with conidial mass on sterile lemmas at<br />
(a) 12X and (b) 30X. Photomicrograph of Pestalotia sp. showing (c) septated conidia with 2–3 hyaline appendages<br />
(40X).<br />
73
→<br />
→<br />
→<br />
→<br />
→<br />
a<br />
b<br />
→<br />
d<br />
e<br />
c<br />
Fig. 90. Habit character of Phaeoseptoria sp. on sterile lemmas at (a) 10X, (b) 25X, and (c) 50X. Photomicrograph<br />
of Phaeoseptoria sp. showing (d) portion of pycnidia and (e) conidia at 40X.<br />
a<br />
b<br />
d<br />
c<br />
e<br />
Fig. 91. Habit character of Phaeotrichoconis crotalariae (Salam & Rao) Subram. on (a) palea and lemma (25X), (b)<br />
sterile lemmas (40X), and (c) awn area (40X). Photomicrograph of P. crotalriae showing (d) portion of conidiophore<br />
(40X) and (e) conidia with large dark brown scar at the base (40X).<br />
74
a<br />
b<br />
d<br />
c<br />
e<br />
Fig. 92. Habit character of Pithomyces sp. on (a) whole seed (9X) and palea and lemma at (b) 18X and (c) 40X.<br />
Photomicrograph of Pithomyces sp. showing (d) mycelia and (e) conidia at 40X.<br />
b<br />
a<br />
f<br />
e<br />
c<br />
d<br />
Fig. 93. Habit character of Pyrenochaeta sp. showing dark and globose pycnidia with bristles on (a) whole seed<br />
(9X) and palea at (b) 25X and 40X. Photomicrograph of Pyrenochaeta sp. showing portion of (d) pycnidia, (e)<br />
bristles, and (f) 1-celled conidia at 40X.<br />
75
→<br />
a<br />
g<br />
→<br />
→<br />
f<br />
g<br />
→<br />
→<br />
b<br />
→<br />
e<br />
→<br />
c<br />
d<br />
Fig. 94. Habit character of Rhizopus sp. showing gray sporangia on (a) whole seed (9X), (b) lemma (25X), and (c)<br />
embryonal area (40X). Photomicrograph of Rhizopus sp. showing (d) rhizoids, (e) sporangiophores, (f) sporangium,<br />
and (g) sporangiospores (10X).<br />
→<br />
→<br />
→ →<br />
→<br />
a<br />
→<br />
b<br />
→<br />
→<br />
c<br />
d<br />
Fig. 95. Habit character of Septogloeum sp. on sterile lemmas at (a) 10X, (b) 25X, and (c) 50X.<br />
Photomicrograph of Septogloeum sp. showing (d) conidia at 40X.<br />
76
→<br />
→<br />
→<br />
→<br />
a<br />
b<br />
e<br />
f<br />
→<br />
c<br />
d<br />
Fig. 96. Habit character of Sordaria fimicola (Roberge ex Desmaz.) Ces. at (a) 9X, (b) 25X, and (c) 50X.<br />
Photomicrograph of S. fimicola showing (d) perithecium and (e) ascus with ascospores at 10X. (f) Ascus with<br />
ascospores at 40X.<br />
a<br />
b<br />
d<br />
c<br />
Fig. 97. Habit character of Spinulospora pucciniiphila Deighton on (a) whole seed (10X), (b) sterile lemma area<br />
(25X), and (c) embryonal side (50X). Photomicrograph of S. pucciniiphila showing (d) bulbils (40X).<br />
77
→<br />
→<br />
→<br />
→<br />
a<br />
b<br />
c<br />
d<br />
Fig. 98. Habit character of Sterigmatobotrys macrocarpa (Corda) Hughes on (a) whole seed (10X), (b) portion of<br />
sterile lemmas (40X), and (c) awn portion (40X). Photomicrograph of S. macrocarpa showing (d) conidia at 40X.<br />
→<br />
a<br />
b<br />
c<br />
d<br />
Fig. 99. Habit character of Taeniolina sp. on sterile lemmas at (a) 12X, (b) 25X, and (c) 40X. Photomicrograph of<br />
Taeniolina sp. showing (d) multiseptate conidia (40X).<br />
78
a<br />
b<br />
c<br />
d<br />
Fig. 100. Habit character of Tetraploa aristata Berk. & Br. on (a) whole seed (12X), (b) palea and lemma (25X), and<br />
(c) palea (50X). Photomicrograph of T. aristata showing (d) conidia with septate appendages (40X).<br />
a<br />
b<br />
c<br />
d<br />
Fig. 101. Habit character of Trichoderma sp. on sterile lemma and palea and lemma at (a) 10X, (b) 25X, and (c) 40X.<br />
Photomicrograph of Trichoderma sp. showing (d) conidia borne in small terminal clusters (40X).<br />
79
a<br />
b<br />
e<br />
c<br />
e<br />
d<br />
Fig. 102. Habit character of Trichothecium sp. on (a) whole seed (9X), (b) embryonal area (25X), and (c) lemma<br />
(50X). Photomicrograph of Trichothecium sp. showing (d) conidiophore and (e) conidia at 40X and stained with<br />
lactophenol blue.<br />
a<br />
b<br />
→→<br />
e<br />
c<br />
d<br />
Fig. 103. Habit character of Tritirachium sp. on (a) whole seed (10X), (b) palea and lemma (18X), and (c) awn (50X).<br />
Photomicrograph of Tritirachium sp. showing (d) branched conidiophore and (e) conidia at 40X.<br />
80
→<br />
→<br />
→<br />
→<br />
→<br />
→<br />
a<br />
→<br />
→<br />
→<br />
b<br />
d<br />
d<br />
c<br />
Fig. 104. Habit character of Ulocladium botrytis Preuss. at (a) 30X and (b) 50X. Photomicrograph of U. botrytis<br />
showing (c) conidiophores and (d) conidia at 40X.<br />
81
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