Fungal Diversity (2018) 90:1–84
https://doi.org/10.1007/s13225-018-0398-4
(0123456789().,-volV)(0123456789().,-volV)
Biodiversity of fungi on Vitis vinifera L. revealed by traditional
and high-resolution culture-independent approaches
Ruvishika S. Jayawardena1,2,3 • Witoon Purahong4 • Wei Zhang1,3 • Tesfaye Wubet4,5 • XingHong Li1,3
Mei Liu1,3 • Wensheng Zhao6 • Kevin D. Hyde2 • JianHua Liu1 • Jiye Yan1,3
•
Received: 17 November 2017 / Accepted: 26 February 2018 / Published online: 14 March 2018
Ó The Author(s) 2018
Abstract
This study is unique as it compares traditional and high-resolution culture-independent approaches using the same set of
samples to study the saprotrophic fungi on Vitis vinifera. We identified the saprotrophic communities of table grape (Red
Globe) and wine grape (Carbanate Gernischet) in China using both traditional and culture-independent techniques. The
traditional approach used direct observations based on morphology, single spore isolation and phylogenetic analysis
yielding 45 taxa which 19 were commonly detected in both cultivars. The same set of samples were then used for Illumina
sequencing which analyzed ITS1 sequence data and detected 226 fungal OTUs, of which 176 and 189 belong to the
cultivars Carbanate Gernischet and Red Globe, respectively. There were 139 OTUs shared between the two V. vinifera
cultivars and 37 and 50 OTUs were specific to Carbanate Gernischet and Red Globe cultivars respectively. In the Carbanate
Gernischet cultivar, Ascomycota accounted for 77% of the OTUs and in Red Globe, almost all sequenced were
Ascomycota. The fungal taxa overlap at the genus and species level between the traditional and culture-independent
approach was relatively low. In the traditional approach we were able to identify the taxa to species level, while in the
culture-independent method we were frequently able to identify the taxa to family or genus level. This is remarkable as we
used the same set of samples collected in China for both approaches. We recommend the use of traditional techniques to
accurately identify taxa. Culture-independent method can be used to get a better understanding about the organisms that are
present in a host in its natural environment. We identified primary and secondary plant pathogens and endophytes in the
saprotrophic fungal communities, which support previous observations, that dead plant material in grape vineyards can be
the primary sources of disease. Finally, based on present and previous findings, we provide a worldwide checklist of 905
fungal taxa on Vitis species, which includes their mode of life and distribution.
Keywords Checklist Grapevine Mycobiome Next generation sequencing Pathogens Saprotrophs
Introduction
Vitis (family Vitaceae) is a plant genus that includes the
economically important grapes, and thus because of its
importance, its pathogens have received a considerable
Electronic supplementary material The online version of this article
(https://doi.org/10.1007/s13225-018-0398-4) contains supplementary
material, which is available to authorized users.
Ruvishika S. Jayawardena, Witoon Purahong and Wei Zhang have
equally contributed to this study.
& Jiye Yan
jiyeyan@vip.163.com
amount of attention during the past decade (Yan et al.
2015; Chethana et al. 2017). The importance of this fruit is
associated with its multiple uses; as a source of nutrition,
health and medicinal value, as well as its high economical
significance (Dohadwala and Vita 2009; Bokulich et al.
2014). About 90% of cultivated grapes in the world are V.
vinifera, which comprises wine, as well as table grapes.
This genus comprises 79 accepted species of perennial
woody and herbaceous vines. There are thousands of cultivars of V. vinifera that has been grown successfully
around the globe (Terral et al. 2009). Species of Vitis are
valued for their decorative foliage providing ornamental
value for the genus. Their ability to cover walls and arches,
as well as providing shade has made them important in
domestic cultivation.
Extended author information available on the last page of the article
123
2
Numerous diseases of grapes have been identified which
reduce the yield and quality of this fruit crop (Úrbez-Torres
et al. 2009). Among various pathogens known on grapevine, the damage caused by fungi is significant (ÚrbezTorres 2011). Most studies on fungal pathogens in grape
have focused on their pathogenic phase, which relies on
direct observation and isolations of fungal pathogens from
infected grape material. Fungi that may live within the host
tissue are known as endophytes and are considered to cause
symptomless infections (Lane and Kirk 2012). Plant
pathogenic fungi can survive by changing their biotrophic
mode from pathogenic to saprotrophic or at least can
remain dormant on the decaying plant materials and
become active when suitable conditions for infection exist
(Hoppe et al. 2016; Purahong et al. 2018). For example,
Botrytis cinerea causing gray mold disease in grape is able
to live as a parasite in green tissues and as a saprotroph in
dead plant material (Armijo et al. 2016). Unfortunately, our
knowledge on saprotrophic fungal community associated
with V. vinifera is limited, especially those obtained by
high-resolution culture-independent techniques. The percentage of potential fungal pathogens hidden in saprotrophic community is still unclear.
Saprotrophs are organisms that derive nourishment from
dead or decaying organic matter (Hyde et al. 2007).
Saprotrophs are heterotrophic organisms that break down
the complex compounds of dead organisms (Deighton
2016). They play an important role as decomposers of dead
organic matter in natural ecosystems by releasing enzymes
from hyphal tips (Duarte et al. 2006; Bucher et al. 2004).
Saprotrophic fungi can be either macrofungi (Agaricus sp.,
Phallus sp.) (Garcı́a et al. 1998) or microfungi (Aspergillus
sp., Dothiorella sp., Mucor sp., Neomassaria sp., Rhizopus
sp.) (Vohnı́k et al. 2011; Hyde et al. 2016). Hyde et al.
(2007) and Purahong et al. (2018), provided evidence that
some plants accommodate large numbers of saprotrophic
taxa and that some might be host- or organ-specific. Other
than being decomposers, saprotrophs can also provide
other eco-system services, such as soil formation, defence
against pathogens, as a food source and modification of
pollutants (Deighton 2016). Promputtha et al. (2007, 2010)
provided evidence that not only fungal pathogens, but also
fungal endophytes, can switch lifestyles to saprotrophs.
Thus, the study of saprotrophic fungal communities associated with V. vinifera can provide information on strict
saprotrophism as well as potential endophytes and pathogens with saprotrophic ability.
Fungal species identification has traditionally been
based on direct observation, microscope examination,
culture dependent isolation and phylogenetic analysis (Cai
et al. 2011; Hyde et al. 2010, 2017; Rastogi and Sani 2011;
Fadrosh et al. 2014, Tibpromma et al. 2017). Such studies
have investigated the microbial ecology of various
123
Fungal Diversity (2018) 90:1–84
environments (Rastogi and Sani 2011). However, it has
been recognized that the actual number of microbes in
nature, often exceed the number of microbes identified by
traditional methods (Fadrosh et al. 2014). Traditional
approaches rely on growing the organisms in media, but
many of the microbes in the environment may not be
cultivatable (Stewart 2012). Artificial medium typically
allows growth of only a small fraction of, often fast
growing organisms. Therefore, traditional techniques do
not provide a total community resolution (Hoppe et al.
2016).
During the past decade, microbial research made a shift
from phylogenetic analyses to experimental characterization of communities through the use of complex experimental designs (Kozich et al. 2013). This shift focused on
relatively inexpensive next-generation sequencing approaches (NGS) and powerful bio-informatics tools to analyse
the microbial ecology (Carraro et al. 2011; Rastogi and
Sani 2011). High-throughput DNA sequencing allows us to
understand the presence of microbes and how their communities are structured in complex ecosystems. Microbiome analysis is a culture-independent technique which
requires a low quantity of sample, but with a high
sequencing depth. The term microbiome refers to the entire
habitat including the microorganisms, their genomes and
the surrounding environment. It is characterized by the
application of one or combinations of metagenomics,
metabonomics, metatranscriptomics and metaproteomics
(Marchesi and Ravel 2015). Analysis of the plant microbiome involves linking microbial ecology and the plants
biology and functions, and at the same time viewing
microorganisms as a reservoir of additional genes and
functions for their host (Vandenkoornhuyse et al. 2015).
Mycobiome refers to the fungal component in a habitat
(Underhill and Iliev 2014). However, these techniques may
also have disadvantages. For example, the conditions that
we select to do the PCR can give us biased results.
Sometimes it is difficult to understand whether the fungi
identified by this technique actually exist in the natural
system (Mitchell and Zuccaro 2006). Therefore, in order to
obtain a better resolution in species identification, richness
and distribution patterns of microbes, a combination of
both approaches (i.e. traditional and culture-independent)
are needed. However, we are aware of no studies that have
been conducted using both these approaches.
There have been many studies of major pathogens from
Vitis using both morphology and phylogeny (Úrbez-Torres
et al. 2012, 2013a, b; Dissanayake et al. 2015; Jayawardena
et al. 2015, 2016a; Chethana et al. 2017). Even though a
number of sexual and asexual fungi have been reported on
Vitis species, updated information of the taxa present in
this genus is lacking. Only some have good illustrations
and gene sequence data. Our knowledge on saprotrophic
Fungal Diversity (2018) 90:1–84
fungal communities associated with V. vinifera is limited
and data based on high-resolution culture-independent
technique is lacking. Besides the percentage of potential
fungal pathogens hidden in saprotrophic community is still
unknown.
In this study, we aim to (i) provide taxonomic information on the saprotrophic microfungi collected from
China, Italy, Thailand and Russia, (ii) compare traditional
and culture-independent approaches for characterizing the
saprotrophic fungal communities associated with two cultivars of V. vinifera in China, (iii) quantify plant pathogens
and endophytes hidden in the saprotrophic fungal community and (iv) provide a worldwide checklist for the fungi
on Vitis species based on previous and current research.
Materials and methods
Study site, sampling and isolation of fungi
Fungal species associated with Vitis sp. were collected
from China (Beijing, Sichuan and Yunnan Province), Italy
(Province of Forlı̀-Cesena), Russia (Rostov Region) and
Thailand (Chiang Sean) (Tables 1, 2). Shoots, leaves,
inflorescences, bark and root samples of Vitis vinifera were
used for isolation. The same set of samples from Beijing
(Red Globe cultivar) and Yunnan Province (Carbanate
Gernischet cultivar) were used for the mycobiome analysis
to establish the fungal communities (Fig. 1). The sample
sets were randomly split into two subsamples to employ the
two approaches at the same time. Specimens were incubated in a moist chamber for 3–7 days at 25 °C, if they did
not sporulate. Fungi were isolated by a modified single
spore/conidial isolation method (Chomnunti et al. 2014)
from the samples. Growth rate, colony characteristics and
sexual/asexual morph morphology were determined from
cultures grown on potato-dextrose agar (PDA) at 25 °C,
under 12 h light/12 h dark. Fungal mycelia and spores
were examined by differential interference contrast (DIC)
and photographed with an axio Imager Z2 photographic
Microscope (Carl Zeiss Microscopy, Germany) (Supplementary Figs. S1a–S1d, S2). Forty conidial measurements
were taken for each isolate. All microscopic measurements
were recorded with ZeM PRo 2012 software. Representative herbariums are deposited in the herbarium of Mae Fah
Luang University, Chiang Rai, Thailand (MFU) and in
Kunming, China (KIB). Representative cultures were
deposited at Mae Fah Luang Culture Collection
(MFLUCC), Beijing Academy of Agriculture and Forestry
Sciences, China (JZB) and Kunming Culture Collection
(KUMCC).
3
DNA extraction, PCR amplification, sequencing
and phylogenetic analysis
The methods used are presented in detail in Jayawardena
et al. (2018).
Culture-independent approach: mycobiome
analysis
Two cultivars were selected for this analysis; Red Globe
being the table grape cultivar and Carbanate Gernischet
being the Wine grape cultivar. Samples of Red Globe (RG)
were collected from Yanqin District of Beijing while
samples of Carbanate Gernischet (CG) were collected from
Yunnan Province were used for this analysis. For each
cultivar, three representative grapevine plants were sampled. The root, bark, shoot, inflorescence and leaves were
homogenized and sub-sampled. For culture-independent
technique of fungal communities, total DNA extraction
was performed using 1 g of ground specimens using 29
CTAB method. All the DNA samples were quantitated and
quality checked with the NanoDrop ND-2000C spectrophotometer (ThermoFisher Scientific, Dreieich, Germany). DNA extracts were then stored at - 20 °C for
further analysis. For fungal Illumina sequencing, we targeted the Internal Transcribed Spacer 1 (ITS1) region of
ribosomal RNA gene cluster. ITS1 was amplified with the
forward primer ITS5-1737 (GGAAGTAAAAGTCGTAACAAGG)
and
reverse
primer
ITS2-2043R
(GCTCGCTTCTTCATCGATGC) (White et al. 1990). The
PCR reaction was performed in a 50 ml volume that contained approximately 10 ng of DNA, ExTaq buffer,
0.2 mM of dNTPs, 0.2 mM of each primer, and 2 units of
ExTaq DNA polymerase. The cycling consisted of an initial denaturing at 94 °C for 30 s, followed by 25 cycles of
denaturing at 94 °C for 30 s, annealing at 54 °C for 1 min
and extension at 72 °C for 2 min, and a final extension at
72 °C for 8 min. All PCR reactions were carried out with
PhusionÒ High-Fidelity PCR Master Mix (New England
Biolabs Inc. Ipswich, MA, USA). The PCR products were
mixed with same volume of 19 loading buffer (contained
SYB green) and then operated electrophoresis on 2%
agarose gel for quality detection. Only samples with bright
main strip between 400–450 bp were chosen for further
experiments. The qualified PCR products were mixed in
equidensity ratios. Then, mixture PCR products were
purified with Qiagen Gel Extraction Kit (Qiagen, Germany) following the manufacture’s protocol.
Sequencing libraries were generated using TruSeqÒ
DNA PCR-Free Sample Preparation Kit (Illumina, San
Diego, CA, USA) following manufacturer’s recommendations and index codes were added. The library quality was
123
4
Table 1 Taxa identified in
China, Russia, Italy and
Thailand by directly observing
specimens
123
Fungal Diversity (2018) 90:1–84
Family
Species
Country
Amorosiaceae
Angustimassarina populi
Italy
Botryosphaeriaceae
Botryosphaeria dothidea
China, Italy
Botryosphaeriaceae
Diplodia seriata
Italy
Botryosphaeriaceae
Dothiorella iberica
Italy
Botryosphaeriaceae
Dothiorella sarmentorum
China, Italy
Botryosphaeriaceae
Neofusicoccum italicum
Italy
Botryosphaeriaceae
Neofusicoccum parvum
Italy
Cantharellales Incertae sedis
Minimedusa sp.
China
Chaetomiaceae
Chaetomium globosum
Italy
Chaetosphaeriaceae
Pseudolachnea hispidula
Italy
Cladosporiaceae
Cladosporium cladosporioides
China, Italy
Cladosporiaceae
Cladosporium cucumerinum
Italy
Diaporthaceae
Diaporthe ampelina
Italy
Diaporthaceae
Diaporthe rudis
Italy
Diaporthaceae
Diatrypaceae
Diaporthe eres
Cryptovalsa ampelina
China
Italy
Didymellaceae
Didymella negriana
Italy
Didymellaceae
Didymella pomorum
China
Didymellaceae
Epicoccum nigrum
Italy
Didymosphaeriaceae
Pseudocamarosporium propinquum
Italy
Glomerellaceae
Colletotrichum dematium
Russia
Glomerellaceae
Colletotrichum godetiae
Italy
Glomerellaceae
Colletotrichum hebeiense
China
Glomerellaceae
Colletotrichum siamense
Italy
Glomerellaceae
Colletotrichum viniferum
China
Glomerellaceae
Colletotrichum truncatum
China
Hypocreaceae
Trichoderma atroviride
China
Hypocreaceae
Trichoderma lixii
China
Hypocreaceae
Trichoderma harzianum
China
Hypocreales genera insertae sedis
Alfaria cyperi-esculenti
Italy
Hypocreales genera insertae sedis
Lophiostomataceae
Alfaria vitis
Lophiostoma macrostomum
Italy
Italy
Massariaceae
Neomassaria fabacearum
Italy
Mucoraceae
Actinomucor elegans
China
Mucoraceae
Mucor racemosus
China
Mucoraceae
Mucor circinelloides
China
Mycosphaerellaceae
Pseudocercospora vitis
Thailand
Peniophoraceae
Peniophora sp.
China
Sporocadaceae
Neopestalotiopsis clavispora
China
Sporocadaceae
Neopestalotiopsis vitis
China
Sporocadaceae
Pestalotiopsis chamaeropis
Italy
Sporocadaceae
Pestalotiopsis sp.
Italy
Sporocadaceae
Pseudopestalotiopsis camelliae-sinensis
Italy
Pleosporaceae
Alternaria alternata
China, Italy
Pleosporaceae
Alternaria italic
Italy
Pleosporaceae
Alternaria vitis
Pleosporaceae
Bipolaris maydis
China
China
Pythiaceae
Pythium sp.
China
Saccotheciaceae
Aureobasidium pullulans
Italy
Schizoparmaceae
Coniella vitis
China
Fungal Diversity (2018) 90:1–84
Table 1 continued
5
Family
Species
Country
Sclerotiniaceae
Botrytis cinerea
China
Sporocadaceae
Seimatosporium vitis
Italy
Stachybotryaceae
Albifimbria verrucaria
China
Stachybotryaceae
Albifimbria viridis
China
Teichosporaceae
Floricola viticola
Italy
Aspergillaceae
Aspergillus aculeatus
China
Aspergillaceae
Aspergillus niger
China
Aspergillaceae
Penicillium brevicompactum
China
Aspergillaceae
Penicillium citrinum
China
Aspergillaceae
Penicillium terrigenum
China
Rhizopodaceae
Rhizopus oryzae
China
Trichocomaceae
Talaromyces amestolkiae
China
Trichocomaceae
Talaromyces pinophilus
China
Trichocomaceae
Talaromyces purpureogenus
China
Xylariaceae
Neoanthostomella viticola
Italy
assessed on the QubitÒ 2.0 Fluorometer (Thermo Scientific) and Agilent Bioanalyzer 2100 system. At last, the
library was sequenced on an IlluminaHiSeq2500 platform
and 250 bp paired-end reads were generated.
Paired-end reads were assigned to samples based on
their unique barcode and truncated by cutting off the barcode and primer sequence. Paired-end reads were merged
using FLASH (V1.2.7, http://ccb.jhu.edu/software/FLASH/
) (Magoč and Salzberg 2011). Quality filtering on the raw
tags was performed under specific filtering conditions to
obtain the high-quality clean tags (Bokulich et al. 2013)
according to the QIIME (V1.7.0, http://qiime.org/index.
html) quality controlled process (Caporaso et al. 2010).
The tags were compared with the reference database (Unite
Database, https://unite.ut.ee/) using UCHIME algorithm
(UCHIME Algorithm, http://www.drive5.com/usearch/
manual/uchime_algo.html) to detect chimera sequences
(Edgar et al. 2011), and then the chimera sequences were
removed (Haas et al. 2011). Then the Effective Tags were
finally obtained. Sequences analysis was performed by
Uparse software (Uparse v7.0.1001, http://drive5.com/
uparse/) (Edgar 2013). Sequences with C 97% similarity
were assigned to the same OTUs. Representative sequence
for each OTU was screened for further annotation. For each
representative sequence, the Unite Database (https://unite.
ut.ee/) (Kõljalg et al. 2013) was used to annotate taxonomic
information based on Blast algorithm, which was calculated by QIIME software (Version 1.7.0) (http://qiime.org/
scripts/assign_taxonomy.html). In order to study phylogenetic relationship of different OTUs, and the difference of
the dominant species in different samples (groups), multiple sequence alignment were conducted using the MUSCLE software (Version 3.8.31, http://www.drive5.com/
muscle/) (Edgar 2004).
All OTU abundance information was normalized using a
standard of sequence number corresponding to the sample
with the least sequences (45, 246 sequences). From the data
set, rare OTUs (singletons), which could have potentially
originated from sequencing errors (Kunin et al. 2010), were
removed. We used a Mantel test based on Bray–Curtis
distance measure with 999 permutations to assess the
correlation between the whole matrix and a matrix
excluding the rare OTUs (Hammer et al. 2001; Hoppe et al.
2016). The results indicated that the removal of rare OTUs
from the fungal communities had no effect (RMantel= 1.000, P = 0.002). Subsequent analysis of alpha diversity and community composition were all performed basing
on these normalized rare OTUs removal data. The fungal
ITS rDNA genes Illumina sequencing data are deposited in
the NCBI under the BioProject No PRJNA437133.
Statistical analysis
Mycobiome analysis
All datasets related to fungal OTU richness were tested for
normality and equality of variances using the Jarque–Bera
test. To assess the coverage of the sequencing depth,
individual rarefaction analysis was performed for each
sample using the ‘‘diversity’’ function in PAST (Hammer
et al. 2001). In this work we used observed fungal OTU
richness and Shannon diversity index as the measures for
fungal diversity. The difference in fungal OTU richness
between the two deadwood species was compared using a
two-sample t test in PAST. To visualize the fungal community compositions, we used non-metric multidimensional scaling (NMDS) analysis based on the Bray–Curtis
dissimilarity index calculated PAST. Similarity
123
6
Fungal Diversity (2018) 90:1–84
Table 2 Taxa identified from the two grape cultivars and their life modes using the traditional approach
Species
Family
Life Mode
References
Actinomucor elegans
var. meitauzae
Mucoraceae
Saprotroph
Zheng and Liu (2005)
Albifimbria viridis
Stachybotryaceae
Saprotroph
Lombard et al. (2016)
Albifimbria verrucaria
Stachybotryaceae
Saprotroph
Lombard et al. (2016)
Alternaria alternata
Pleosporaceae
Pathogen, endophyte,
saprotroph
French (1989), Mulenko et al. (2008), Kakalikova et al.
(2009), Gonzalez and Tello (2011)
Alternaria vitis
Pleosporaceae
Pathogen, endophyte,
saprotroph
Zhang (2003), Zhuang (2005)
Aspergillus aculeatus
Aspergillaceae
Secondary pathogen,
saprotroph
Jarvis and Traquair (1984)
Aspergillus niger
Aspergillaceae
Secondary pathogen,
endophyte, saprotroph
Bobev (2009), Casieri et al. (2009), Gonzalez and Tello
(2011)
Bipolaris maydis
Pleosporaceae
Saprotroph
Manamgoda et al. (2014)
Botryosphaeria
dothidea
Botryosphaeriaceae
Pathogen, endophyte,
saprotroph
Úrbez-Torres et al. 2012, 2013a, b
Botrytis cinerea
Sclerotiniaceae
Pathogen
Piqueras et al. (2014), Saito et al. (2016)
Cladosporium
cladosporioides
Cladosporiaceae
Pathogen, endophyte,
saprotroph
Swett et al. (2016)
Cladosporium sp.
Cladosporiaceae
Pathogen, endophyte,
saprotroph
Swett et al. (2016)
Clonostachys rosea
Bionectriaceae
Pathogen, endophyte,
saprotroph
Casieri et al. (2009)
Colletotrichum
hebeiense
Glomerellaceae
Pathogen
Yan et al. (2015)
Colletotrichum
truncatum
Glomerellaceae
Pathogen
Pan et al. (2016)
Colletotrichum
viniferum
Glomerellaceae
Pathogen
Peng et al. (2013)
Coniella vitis
Schizoparmaceae
Pathogen
Chethana et al. (2017)
Diaporthe eres
Diaporthaceae
Pathogen
Bastide et al. (2017)
Didymella pomorum
Didymellaceae
Saprotroph
Cook and Dubé (1989)
Dothiorella
sarmentorum
Botryosphaeriaceae
Pathogen
Carlucci et al. (2015)
Epiccocum nigrum
Didymellaceae
Saprotroph
Casieri et al. (2009)
Exserohilum rostratum
Pleosporaceae
Saprotroph
Ariyawansa et al. (2015)
Fusarium oxysporum
Nectriaceae
Pathogen
Gonzalez and Tello (2011)
Fusarium sp.
Nectriaceae
Pathogen
Gonzalez and Tello (2011)
Minimedusa sp.
Cantharellales
incertae sedis
Saprotroph
Beale and Pitt (1990)
Mucor racemosus
Mucoraceae
Secondary pathogen
Gonzalez and Tello (2011)
Mucor circinelloides
Mucoraceae
Secondary pathogen
Gonzalez and Tello (2011)
Neopestalotiopsis
clavispora
Sporocadaceae
Saprotroph
Maharachchikumbura et al. (2015)
Neopestalotiopsis vitis
Sporocadaceae
Pathogen
Jayawardena et al. (2015, 2016a, b)
Paraphoma
chrysanthemicola
Pleosporales
incertae sedis
Saprotroph
Hofstetter et al. (2012)
Penicillium
brevicompactum
Aspergillaceae
Secondary pathogen
Kim et al. (2007)
Penicillium citrinum
Aspergillaceae
Secondary pathogen
Kim et al. (2007)
Penicillium terrigenum
Aspergillaceae
Kim et al. (2007)
Torrejón (2013)
Weber et al. (2004)
Peniophora sp.
Peniophoraceae
Secondary pathogen
Saprotroph
Phoma medicaginis
Didymellaceae
Saprotroph
123
Fungal Diversity (2018) 90:1–84
7
Table 2 (continued)
Species
Family
Life Mode
References
Pythium amasculinum
Pythiaceae
Pathogen
Uzuhashi et al. (2010)
Rhizopus oryzae
Rhizopodaceae
Secondary pathogen
Gonzalez and Tello (2011)
Septoriella allojunci
Dothideomycetes
incetae sedis
Saprotroph
Li et al. (2015)
Stagonosporopsis sp. 1
Stagonosporopsis sp.2
Didymellaceae
Didymellaceae
Saprotroph
Saprotroph
Hofstetter et al. (2012)
Hofstetter et al. (2012)
Talaromyces pinophilus
Trichocomaceae
Saprotroph
Yilmaz et al. (2014)
Talaromyces
purpurogenus
Trichocomaceae
Saprotroph
Yilmaz et al. (2014)
Talaromyces
amestolkiae
Trichocomaceae
Saprotroph
Yilmaz et al. (2014)
Trichoderma atroviride
Hypocreaceae
Saprotroph
Gonzalez and Tello (2011)
Trichoderma harzianum
Hypocreaceae
Saprotroph
Gonzalez and Tello (2011)
Trichoderma lixii
Hypocreaceae
Saprotroph
Gonzalez and Tello (2011)
Percentages (SIMPER) analysis using PAST was used to
obtain the identity and relative abundances of the fungal
taxa that contributed to 92.92% of the observed pair-wise
variation in the fungal community composition due to
different V. vinifera cultivars. To accounting for the effect
of locations when compared the fungal community compositions of the two grape cultivars which were collected
from different locations, we eliminated all location specific
fungal OTUs (87 OTUs). We finally retained 139 OTUs for
the community composition analysis using NMDS based
on the Bray–Curtis dissimilarity. The results from these
reduced datasets were highly consistent compared with the
total datasets (Supplementary Fig. S3a, b). Potential fungal
functional groups were identified using the online Guilds
application tool: FUNGuildb (Nguyen et al. 2015). The
ITS1 fragments were extracted from both the Sanger
sequencing (traditional) and Illumina sequencing datasets
using ITS1. The output showed that both datasets have the
ITS1 region except culture sequences of the genus
Neopestalotiopsis (9 sequences). The sequence similarity
based comparison was performed using the cd-hit-est-2d
algorithm at 90% similarity level for a genus level
comparison.
Percent occurrence of a taxon A (%)
Occurrence of taxon A
¼
100
Occurrence of all taxa in one sample
Species richness
¼ the number of different species represented in an
ecological community
Following diversity indices were calculated using the R
software for the two cultivars and the habits.
(i)
Shannon Wiener’s Index (H) ¼
X
pi ln pi ;
where pi is the frequency of fungal species I occurring on a specific sample (Begon et al. 1993;
Wong and Hyde 2001; Wang et al. 2008).
(ii)
Srensen’s index of similarity (S)
¼ 2c=ða þ bÞ;
where a is the total number of species on host A,
b is the total number of species on host B and c is
the number of species on both host. Similarity is
expressed with values between 0 (no similarity)
and 1 (absolute similarity) (Wang et al. 2008).
Diversity analysis
Taxa were recorded as either present or absent from each
sample. Occurrence of a fungus was designated based on
the presence of a particular fungus on the host samples.
Percentage occurrence of a taxon on one sample was calculated using the following formula (Tsui et al. 2001;
Yanna and Hyde 2002; Wang et al. 2008):
Compiling the checklist
The checklist is based on, articles in referred journals,
Index to Saccardo’s Sylloge fungorum, Petrak’s Lists,
Index of Fungi, graduate student theses, books, and webbased resources such as annual reports on this host and the
SMML database (https://nt.ars-grin.gov/fungaldatabases/)
123
8
Fungal Diversity (2018) 90:1–84
Fig. 1 Dead V. vinifera samples
at collection sites
(latest accessed 14-9-2017). The mode of life, such as
pathogen, endophyte or saprotroph is listed. The checklist
includes species names, family, life modes, disease name if
any and locality. The current name is used according to
Index Fungorum (2018) and Wijayawardene et al. (2017)
and the classification follows Wijayawardene et al. (2018).
Genera and species are listed in alphabetical order. Identification confirmed by molecular data is marked with an
asterisk (*). In some cases, the host name given in the
original citation was changed to be consistent with current
taxonomy. In a few cases, neither the species cited nor a
proper synonym was identified and the species name was
used as originally cited.
123
Results
Species identified from fresh collections based
on morphology and phylogeny (traditional
method)
Fungal saprophytic diversity and community composition
of the two grape cultivars: traditional method
Examination of decaying leaves, shoots, inflorescence, berries, root and bark of two cultivars of V. vinifera from China
yielded 461 collections for the Red Globe variety and 180
collections for Carbanate Gernischet. The Red Globe variety
Fungal Diversity (2018) 90:1–84
9
had higher species richness (41) than the Carbanate Gernischet variety (23), however the Shannon diversity was not
significantly different (Table 3). The majority of the culturable saprotrophic fungi were ascomycetes. However, there
were two species belonging to Agaricomycetes and one species belonging to Oomycota incertae sedis. Thirty genera and
45 taxa were identified based on morphology and phylogenetic sequence data. From the identified isolates, 32.6% were
Sordariomycetes, 26.1% Dothideomycetes 19.7% Eurotiomycetes, 6.5% Mucoromycetes, 4.4% Agaricomycetes,
2.2% Leotiomycetes and 2.2% of Oomycota incertae sedis.
There were four taxa belonging to Zygomycota incertae sedis,
which we were unable to identify. The identified Sordariomycetes belonged to Bionectriaceae (6.7%), Diaporthaceae
(6.7%), Glomerellaceae (20%), Hypocreaceae (20%), Nectriaceae (13.3%), Schizoparmaceae (6.7%), Stachybotryaceae (13.3%) and Sporocadaceae (13.3%). Dothideomycete
isolates belonged to Botryosphaeriaceae (16.7%), Cladosporiaceae (16.7%), Didymellaceae (33.3%) and
Pleosporaceae (33.3%). The rest of the isolates belong to
Mucoraceae (6.5%), Peniophoraceae (2.2%), Pythiaceae
(2.2%), Rhizopodaceae (2.2%), Sclerotiniaceae (2.2%) and
Trichocomaceae (17.4%). Among those 45 taxa, we found 19
species that were common on both cultivars: Actinomucor
elegans, Alternaria alternata, Aspergillus niger, A. aculeatus,
Cladosporium cladosporioides, Cladosporium sp., Clonostachys rosea, Coniella vitis, Diaporthe eres, Fusarium oxysporum, Mucor racemosus, Penicillium terrigenum, Phoma
medicaginis, Rhizopus oryzae, Talaromyces amestolkiae, T.
pinophilus, T. purpurogenus and T. harzianum. The Sørensen’s index of similarity of the two grape cultivars was 0.58.
We have identified 45 taxa to species level, although in six
cases the identification is only to genus level due to lack of
enough molecular data. Taxa were identified using both
morphology and molecular techniques. Identified species are
listed in Tables 1 and 2 (Supplementary Figs. S1a–d, S2).
Fungal saprophytic diversity and community
composition of the two grape cultivars: cultureindependent technique
Bioinformatics processing of the sequence data sets
A total of 638,146 quality-filtered fungal ITS reads were
obtained after removal of chimeric and the unique tag
Table 3 Richness and diversity (mean ± SD, n = 3) of fungi
detected in the two Vitis vinifera cultivars
RG
CG
Species richness
41
23
Shannon
2.5433 ± 0.251
2.4743 ± 0.187
(3703 sequences) sequences. After normalizing all data sets
to a smallest sequence read (45, 246 sequences) and
removing all rare taxa, the final analyse data sets contained
226 fungal OTUs. Phylogenetic trees for the top 20 species
in different samples of the two cultivars Carbanate Gernischet and Red Globe of Vitis vinifera are given in Fig. 2.
With the high number of sequence reads per sample
obtained in this study, the sample-based rarefaction curves
almost reached saturation for all samples (Fig. 3a). We
used the observed OTU richness and Shannon diversity
directly for further analyses.
Fungal saprotrophic OTU diversity and distribution
in the two cultivars of Vitis vinifera
Diverse fungi colonized the debris samples derived from
Carbanate Gernischet and Red Globe cultivars. Fungal OTU
richness was not significantly different between the two V.
vinifera cultivars tested in this study, ranging from 122–137
(127.33 ± 4.84 (mean ± SD); Carbanate Gernischet) and
116–141 (126.33 ± 7.54 (mean ± SD); Red Globe)
(t = 0.11, P = 0.916). Shannon diversity also showed a similar trend ranging from 1.98–2.35 (2.16 ± 0.11 (mean ±
SD); Carbanate Gernischet) and 1.78–1.98 (1.86 ± 0.06
(mean ± SD); Red Globe) (t = 2.41, P = 0.07). In total we
detected 226 fungal OTUs with 176 and 189 belonging to the
cultivars Carbanate Gernischet and Red Globe, respectively.
There were 139 Fungal OTUs shared between the two V.
vinifera cultivars and 37 and 50 OTUs were specific to Carbanate Gernischet and Red Globe cultivars. When we took
each replicate into account, we detected only moderate proportion of fungal OTUs shared across different replicates
(31–44%, 51 OTUs, Fig. 3b). Distributions of fungal OTUs
across replicates for the two cultivars and for each specific
cultivar are shown in Fig. 3b–d.
Fungal saprophytic community composition: cultureindependent technique
The NMDS ordination plot and SIMPER analysis revealed
distinct fungal communities in the two cultivars of V.
vinifera samples (Table 4 and Supplementary Fig. S3a, b).
Overall, fungal community composition of the two cultivars had the overall average dissimilarity of 94.29% (based
on Bray–Curtis distance measure) and 30 fungal OTUs
mostly responsible for differences in fungal community
composition were all together accounting for 94.41% of the
overall average dissimilarity (Table 4). The difference in
fungal community composition between the two cultivars
of V. vinifera was detected across different taxonomic
levels (Supplementary Figs. S4, S5).
In Carbanate Gernischet, members of Ascomycota were
commonly detected accounting for 77% (46%
123
10
Fungal Diversity (2018) 90:1–84
Fig. 2 Phylogenetic tree of top 20 species in different samples of the two cultivars Carbanate Gernischet and Red Globe of Vitis vinifera
Sordariomycetes, 19% Eurotiomycetes and 7% Dothideomycetes) of total sequences in this cultivar followed by
unidentified phylum (23%; Fungal OTU-7) and Basidiomycota and Zygomycota (less than 0.1%). In Red Globe,
almost all sequences were assigned to Ascomycota (97%;
51% Eurotiomycetes, 42% Sordariomycetes, and 3%
Dothideomycetes) followed by Basidiomycota (3%; 1%
Agaricomycetes and 1% Tremellomycetes) and unidentified phylum (Fungal OTU-7) and Zygomycota were negligible (altogether less than 0.5%). Phylogenetic tree for the
abundance at genus level using the top 35 genera detected
in the two cultivars are shown in Fig. 4. The difference
between the fungal community composition of the two
123
cultivars of V. vinifera were clearly demonstrated at OTU
level: Trichothecium roseum OTU-1, Fungal-OTU-7,
Aspergillus piperis OTU-5 and Nectriaceae OTU-3 were
commonly detected (10–20%) in Carbanate Gernischet, but
almost absent in Red Globe (represented by Aspergillus
OTU-11, Ilyonectria macrodidyma OTU-4, Aspergillus
cibarius OTU-2 and Diaporthaceae OTU-10; 11–19%;
Table 4).
Using presence/absence data, we found that for both
Vitis vinifera cultivars Ascomycota (Carbanate Gernischet = 151 OTUs and Red Globe = 162 OTUs) was the
richest OTU phylum followed by unidentified phylum,
Basidiomycota (11–14 OTUs) and Zygomycota (2 OTUs).
Fungal Diversity (2018) 90:1–84
11
Fig. 3 Rarefaction curves (a),
and Venn diagrams show
distribution of OTUs across
different samples (1–3): (b) in
both Carbanate Gernischet (CG)
and Red Globe (RG) cultivars,
(c) only Carbanate Gernischet
and (d) only Red Globe
Patterns of the richest OTU classes and orders were similar
for both cultivars: Sordariomycetes (Hypocreales (Carbanate Gernischet = 32 OTUs and Red Globe = 39 OTUs),
Sordariales (Carbanate Gernischet = 13 OTUs and Red
Globe = 13 OTUs), Microascales (Carbanate Gernischet = 10 OTUs and Red Globe = 11 OTUs)], Eurotiomycetes (Eurotiales, Carbanate Gernischet = 41 OTUs
and Red Globe = 38 OTUs) and Dothideomycetes
(Pleosporales, Carbanate Gernischet = 7 OTUs and Red
Globe = 7 OTUs).
Comparing and matching of traditional
and culture-independent approaches
Several commonly detected fungal genera (Aspergillus,
Clonostachys and Fusarium) were detected in both
approaches. However, there are many highly or frequently
detected genera in the mycobiome that were not detected in
the traditional method. These include Acrostalagmus,
Aureobasidium, Ceratobasidium, Chrysosporium, Ilyonectria, Lasiodiplodia, Microascus, and Trichothecium (Supplementary Table S1). Some frequently isolated fungi,
especially the fast growing ones (Rhizopus and Mucor)
were not detected in mycobiome analysis.
ITS sequences obtained from both traditional and
culture-independent methods were compared using the
query and cluster cover. This showed that the saprotrophs
detected from the two approaches are consistent in most
cases. However, in few cases we found inconsistent identifications which have arisen from the lower level of taxonomic assignment in the culture-independent (amplicon
sequencing) as compared with traditional approaches. For
example, Diaporthe eres and Alternaria identified via the
traditional approach were identified as Diaporthaceae and
Pleosporaceae in the culture-independent analyses. A
mismatch was also found between Albifimbria viridis and
Myrothecium sp., which are classified in the same order
(Hypocreales). The sexual morph genus Talaromyces was
matched with its potential asexual morph (Penicillium).
We found that twelve taxa detected from traditional
method form a cluster (91–100% similarity) with 25 fungal
OTUs from the culture-independent methods (Table 5).
We were able to assign 25 OTUs from NGS: 20 OTUs to
genus and 5 OTUs (similarity 99–100%) to species level
respectively (Table 5). We removed two OTUs as singletons (Botryosphaeria OTU-178 and Ascomycota OTU213) as they were detected only once. However, in the
direct matching of ITS sequences, these fungal OTUs
showed 97 and 100% similarity to Botryospaeria dothidea
and Coniella vitis, respectively. The other fungi that we
were able to identify to the species level are Aspergillus
niger, Clonostachys rosea, Botrytis cinerea, and Albifimbria viridis. Most of the frequently detected genera in the
traditional approach (i.e. with relative abundance higher
than 5%; Alternaria, Clonostachys, Fusarium) were also
detected in culture-independent approach. Rhizopus sp. and
123
12
Fungal Diversity (2018) 90:1–84
Table 4 Similarity percentages (SIMPER) analysis showing the top 30 fungal OTUs mostly responsible for differences in fungal community
composition between Carbanate Gernischet(CG) and Red Globe (RG) cultivars; OA Dissimilarity = overall average dissimilarity
Talaromyces sp. were frequently detected in the traditional
approach, but exhibited low relative abundances or disappeared in the culture-independent approach.
Fungal functional groups identified using
traditional and culture-independent approaches
Among the 45 identified taxa based on traditional method,
17 are well known pathogens on V. vinifera causing severe
yield as well as economic loss to viticulture around the
123
world (Table 2). Six species of secondary pathogens of V.
vinifera were also identified in this study. Most of the
pathogens tend to survive or overwinter on dead plant
material as saprotrophs and act as the primary inoculums
once the conditions are favourable (Armijo et al. 2016).
In total, 143 fungal OTUs (63% of total fungal OTUs)
were successfully assigned for their functions (Supplementary Table S1). We identified six functional groups of
fungi associated with dead materials of V. vinifera:
saprotrophs, plant pathogens, endophytes, fungal parasites–
Fungal Diversity (2018) 90:1–84
13
Fig. 4 Abundance phylogenetic
tree at genus level (top 35
genera) in two cultivars
[Carbanate Gernischet (CG1-3)
and Red Globe (RG1-3)] of
Vitis vinifera
saprotrophs (mycoparasites–saprotrophs), ectomycorrhizae
and animal pathogens. The fungal community was dominated by saprotrophs (102 OTUs) and plant pathogens (22
OTUs), which accounted for 71% and 15% of the function
assigned to fungal OTUs in this study. Clonostachys, Lasiodiplodia and Trichothecium, were the most commonly
detected plant pathogen genera with relative abundances
1–10%. Botrytis sp., an important fungal pathogen in
grape, was also detected with low relative abundance.
Endophytes together with endophyte–saprotrophs and
endophyte–plant pathogens (9 OTUs) contributed little and
most OTUs were detected with low relative abundance,
except, Acrostalagmus luteoalbus. All fungal OTUs with
their potential functions are listed in Supplementary
Table S1.
Checklist of fungi on Vitis
Nine-hundred and six fungal taxa have been reported on
Vitis species and are listed in Table 6, although the actual
number of fungal taxa associated with this host is likely
much higher. It is not possible to reconfirm all previous
reports by re-examining collections to confirm their identities. In many cases no fungarium material is linked to the
reports, while examining nearly 900 specimens would be
an almost impossible task. Even if it was were possible, it
would most likely be futile, since molecular data would be
needed to establish correct names. This is extremely difficult based on the presently available techniques and not
permitted by many fungaria. Most of the 905 taxa reported
from Vitis species do not have sequence data. Therefore,
recollecting and sequencing these taxa are essential to
establish and accurate species list associated with Vitis
species.
123
14
Fungal Diversity (2018) 90:1–84
Table 5 Matching of fungal isolates to the saprotrophic mycobiome of Vitis vinifera
Fungal taxon
(culture)
Albifimbria
viridis
Alternaria spp.
Relative abundance
in culture (%)
0.55
28.14
Fungal taxa (mycobiome)
Relative abundance in
mycobiome (%)
Cluster identification
(coverage) %
Number of
OTUs in cluster
Myrothecium
0.010
99 (100)
1
Ampelomyces, Phoma,
Pleosporaceae OTU, Fungal
OTU
0.636
92–100 (95–100)
4
Aspergillus
niger
6.01
Aspergillus
3.683
99 (100)
1
Botryospaeria
dothidea
0.27
Botryospaeria
Remove as singleton
97 (100)
1
Botrytis
cinerea
2.73
Botrytis
0.002
100 (100)
1
Clonostachys
rosea
2.19
Clonostachys
5.244
99 (100)
1
Coniella vitis
1.09
Ascomycota OTU
Remove as singleton
100 (100)
1
Diaporthe eres
1.37
Diaporthaceae OTUs
0.070
92–97 (98–100)
2
Fusarium sp.
Penicillum sp.
25.41
0.54
Fusarium, Nectriaceae OTUs
Penicillium
5.368
0.203
93–100 (83–87)
91–100 (81–100)
8
3
Talaromyces
amestolkiae
5.46
Penicillium
0.001
96 (100)
1
Tricoderma
atroviride
4.09
Tricoderma
0.008
97 (99)
1
Discussion
Before the advent of molecular data in taxonomy, studies
on the fungi on Vitis were based on traditional methodology and have resulted in hundreds of records of fungi from
this host genus (Table 6). Most recent studies have been
related to pathogens that affect grape yield and production
(Úrbez-Torres et al. 2012, 2013a, b; Dissanayake et al.
2015; Liang et al. 2016; Jayawardena et al. 2015, 2016a;
Yan et al. 2015; Chethana et al. 2017) and have resulted in
well-resolved taxonomy as they have used molecular data.
However, studies on saprobes using molecular data and
culture-independent techniques have not been used to
identify the fungi on Vitis to date. In this study, we
therefore provide the first work comparing saprobes on
Vitis sp. using both traditional and culture-independent
approaches, with well-resolved taxonomic identifications
based on molecular analyses. The taxa derived from both
approaches are compared as the same samples were used in
the study. We have also established the saprotrophic
communities associated with both wine and table grapevine
cultivars and demonstrate cultivar specific communities for
each grapevine cultivar. A checklist of fungi of Vitis is also
provided which is an important resource for viticulture.
123
Microfungi collected from China, Italy, Russia
and Thailand
Sixty-seven saprotrophic taxa from 46 genera were identified in this study (Table 1). Using traditional methodology and analyses of molecular data, we identified two new
species, and 41 new host or distribution records for V.
vinifera. Taxonomic details, descriptions, photographic
plates and phylogenetic analyses are provided in
Jayawardena et al. (2018). Some of these genera have a
wide distribution. For example, botryosphaerious and
Colletotrichum taxa have a wide distribution. These taxa
are well-known pathogens and can be spread to other
countries undetectable through the exportation of rootstocks. Some genera are only known from one or two
countries. This may be due to the lack of data on the fungi
associated with this host.
Comparisons of traditional and cultureindependent approaches for characterizing
the saprotrophic fungal communities associated
with two cultivars of Vitis vinifera
Most previous studies on fungi on grapevine have relied on
traditional approaches (Table 6). Some recent identification of isolated taxa have incorporated analyses of ITS
sequence data (Guo et al. 2003; Promputtha et al. 2007),
Fungal Diversity (2018) 90:1–84
15
Table 6 Check list of fungi on Vitis sp. (classification follows Wijayawardene et al. 2017, 2018)
Species
Family
Life
mode
Disease caused
Locality
References
Acremonium acutatum
W. Gams*
Bionectriaceae
P
Unknown
Korea
Oh et al. (2014)
A. alternatum Link*
Bionectriaceae
E
China, Greece, Spain
Pantidou (1973), Benavides
et al. (2013), Dissanayake
et al. (2018)
Acremonium sp.*
Bionectriaceae
P, E
Argentina, China, Iran, Italy,
South Africa, Korea, Spain
Gatica et al. (2001), Halleen
et al. (2003), Luque et al.
(2009), Gonzalez and Tello
(2011), Mohammadi and
Banihashemi (2012),
Mondello et al. (2013), Oh
et al. (2014), This study
Acrocalymma vagum
(D.F. Farr) P.W. Crous
& T.
Trakunyingcharoen*
Acrocalymmaceae
U
Spain
Trakunyingcharoen et al.
(2014)
Acrospermum viticola
Ikata & Hitomi
Acrospermaceae
U
China, Japan, Korea
Tai (1979), Cho and Shin
(2004), Kobayashi (2007)
Acrostalagmus
luteoalbus (Link) Zare,
W. Gams & Schroers*
Actinomucor elegans
(Eidam) C.R. Benj. &
Hesselt*
Plectosphaerellaceae
S
China
This study
Mucoraceae
S
China
This study, Jayawardena et al.
(2018)
Agaricus viticola
Schulzer
Agaricaceae
S
Slavonia
Saccardo (1878)
Albifimbria verrucaria
(Alb. & Schwein.) L.
Lombard & Crous*
Stachybotryaceae
S
China
This study, Jayawardena et al.
(2018)
A. viridis L. Lombard &
Crous*
Stachybotryaceae
S
China
This study, Jayawardena et al.
(2018)
Alfaria cyperi-esculenti
Crous, Montaño-Mata
& Garcı́a-Jim*
Hypocreales genera
incertae sedis
S
Italy
This study, Jayawardena et al.
(2018)
Alfaria vitis
Manawasinghe,
Camporesi & K.D.
Hyde*
Hypocreales genera
incertae sedis
S
Italy
This study, Jayawardena et al.
(2018)
Alternaria lternate (Fr.)
Keissl.*
Pleosporaceae
P, E,
S
Brunei, China, Italy, Poland,
Slovakia, Spain, USA
Peregrine and Ahmad (1982),
French (1987, 1989),
Mulenko et al. (2008),
Kakalikova et al. (2009),
Gonzalez and Tello (2011),
Dissanayake et al. (2018),
This study, Jayawardena
et al. (2018)
A. arborescens E.G.
Simmons*
Pleosporaceae
E
Spain, Switzerland
Casieri et al. (2009), Gonzalez
and Tello (2011)
A. italica J.F.
Li,Camporesi & K.D.
Hyde*
Pleosporaceae
S
Italy
This study, Jayawardena et al.
(2018)
A. tenuissima (Kunze)
Wiltshire
Pleosporaceae
E
Malawi, Spain
Wiehe (1948), Peregrine and
Siddiqi (1972), Gonzalez
and Tello (2011)
‘Hoja de
malvon’
Fruit rot
123
16
Fungal Diversity (2018) 90:1–84
Table 6 (continued)
Species
Family
A. viticola Brunaud
Pleosporaceae
P
Fruit rot
China
Tai (1979)
A. vitis Cavara*
Pleosporaceae
P, S
Leaf blight,
Fruit rot
Chile, China, El Salvador,
Greece, India, Italy, Romania,
Russia, Thailand,
Turkmenistan
Cavara (1888), Makovetz
(1933), Stevenson and
Wellman (1944), Mujica
and Vergara (1945),
Nasyrov (1964), Sarbhoy
et al. (1971), Pantidou
(1973), Giatgong (1980),
Bechet and Sapta-Forda
(1981), Zhang (2003),
Zhuang (2005), This study,
Jayawardena et al. (2018)
A. viniferae Yong Wang
bis, Y.Y. Than, K.D.
Hyde & Xing H. Li*
Pleosporaceae
P
On pedicels and
rachis
China
Tao et al. (2014)
Alternaria sp.*
Pleosporaceae
P, E
On pedicels and
rachis
Cuba, France, Italy, Poland,
South Africa, Spain,
Switzerland, USA
Preston (1945), Harvey
(1955), Arnold (1986), Cook
and Dubé (1989), Larignon
and Dubos (1997), Halleen
et al. (2003), Mulenko et al.
(2008), Casieri et al. (2009),
Gonzalez and Tello (2011),
Mondello et al. (2013)
Amerosporium
concinnum Petr.
Ascomycota genera
incertae sedis
P
Excoriose and
die back
Portugal
Phillips (2000)
Ampelomyces quisqualis
Ces.
Phaeosphaeriaceae
M
South Africa
Doidge (1950)
Ampelomyces sp.*
Phaeosphaeriaceae
S
China
This study
Amphisphaeria sylvan
Sacc. & Speg
Amphisphaeriaceae
S
Italy
Farr (1973)
A. humuli (Fautrey)
Rudakov
Amphisphaeriaceae
M
Ukraine
Dudka et al. (2004)
Angustimassarina populi
Thambug. & K.D.
Hyde*
Amorosiaceae
S
Italy
This study, Jayawardena et al.
(2018)
Aplosporella
beaumontiana S.
Ahmad
Aplosporellaceae
S
India
Rajak and Pandey (1985)
A. fabiformis (Pass. &
Thüm.) Petr. & Syd.
Aplosporellaceae
P
On stem
Italy, Pakistan, USA
Petrak and Sydow (1927),
Anonymous (1960), Ahmad
(1969)
A. japonicas Ellis &
Everh.
Aplosporellaceae
P
On stem
China
Tai (1979)
A. viticola Cooke &
Massee
Aplosporellaceae
P
On stem
UK
Saccardo (1878)
Aplosporella sp.*
Aplosporellaceae
S
China
This study
Apodus sp.*
Lasiosphaeriaceae
S
China
This study
Arachnomyces sp.*
Arachnomycetaceae
S
China
This study
Armillaria limonea (G.
Stev.) Boesew
Physalacriaceae
P
Root rot
New Zealand
Gadgil (2005)
A. luteobubalina Watling
& Kile
Physalacriaceae
P
Root rot
Australia
Cook and Dubé (1989)
123
Life
mode
Disease caused
Locality
References
Fungal Diversity (2018) 90:1–84
17
Table 6 (continued)
Species
Family
Life
mode
Disease caused
Locality
References
A. mellea (Vahl) P.
Kumm.
Physalacriaceae
P
Root rot
Australia, Greece, Italy, Japan,
Scotland, USA
Anonymous (1960), Foister
(1961), Simmonds (1966),
French (1989), Zervakis
et al. (1998), Holevas et al.
(2000), Kobayashi (2007),
Bobev (2009), Prodorutti
et al. (2009)
A. novae-zelandiae (G.
Stev.) Boesew
Physalacriaceae
P
Root rot
New Zealand
Gadgil (2005)
Armillaria sp.
Physalacriaceae
P
Root rot
Australia, New Zealand
Pennycook (1989), Shivas
(1989)
Arthrobotrys sp.*
Orbiliaceae
S
Switzerland
Casieri et al. (2009)
Arthrographis sp.*
Eremomycetaceae
S
China
This study
Arthrinium arundinis*
(Corda) Dyko & B.
Sutton
Apiosporaceae
E
Switzerland
Casieri et al. (2009)
A. phaeospermum
(Corda) M.B. Ellis
Apiosporaceae
E
Spain
Gonzalez and Tello (2011)
A. rasikravindrae Shiv
M. Singh, L.S. Yadav,
P.N. Singh, Rah.
Sharma & S.K. Singh*
Apiosporaceae
E
China
Dissanayake et al. (2018)
Arthrinium sp.
Apiosporaceae
U
Russia
Melnik and Popushoi (1992)
Arxiomyces vitis (Fuckel)
P.F. Cannon & D.
Hawksw.
Ceratostomataceae
U
Europe, Poland
von Arx and Mueller (1954),
Mulenko et al. (2008)
Ascochyta ampelina
Sacc.
Didymellaceae
P
Greece, Pakistan, Romania,
UK, USA
Saccardo (1878), Anonymous
(1960), Pantidou (1973),
Ahmad et al. (1997), Jones
and Baker (2007)
Ascorhizoctonia sp.*
Pyronemataceae
E
China
Dissanayake et al. (2018)
Aspergillus aculeatus
Iizuka*
Aspergillaceae
P, S
Bunch rot
Canada, China
Jarvis and Traquair (1984),
This study, Jayawardena
et al. (2018)
A. carbonarius (Bainier)
Thom*
Aspergillaceae
P
Bunch rot
South Africa, USA
Setati et al. (2015), RooneyLatham et al. (2008)
A. cibarius S.B. Hong &
Samson*
Aspergillaceae
S
China
This study
A. flavus Link
A. glaucus (L.) Link
Aspergillaceae
Aspergillaceae
P
U
Italy
Dominican Republic
Greuter et al. (1991)
Ciferri (1929, 1961)
A. aponicas Saito*
Aspergillaceae
E
China
Dissanayake et al. (2018)
A. niger Tiegh.*
Aspergillaceae
P, E,
S
Australia, Bulgaria, China,
Cyprus, Italy, Japan, Spain,
South Africa, Switzerland,
USA, Zimbabwe
Georghiou and Papadopoulos
(1957), Whiteside (1966),
Cook and Dubé (1989),
Setati et al. (2015),
Michailides et al. (2002),
Kobayashi (2007), Vitale
et al. (2008), Bobev (2009),
Casieri et al. (2009),
Gonzalez and Tello (2011),
Dissanayake et al. (2018),
This study, Jayawardena
et al. (2018)
On leaves
Bunch rot
Bunch rot,
Canker
123
18
Fungal Diversity (2018) 90:1–84
Table 6 (continued)
Species
Family
Life
mode
A. terreus Thom*
Aspergillaceae
E, S
Disease caused
Canker
Locality
References
Spain, China
Gonzalez and Tello (2011),
This study
A. tubingensis Mosseray*
Aspergillaceae
P
Spain
Garcia-Benavides et al. (2013)
A. piperis Samson &
Frisvad*
Aspergillaceae
S
China
This study
A. pseudodeflectus
Samson & Mouch.*
Aspergillaceae
E, S
China
Dissanayake et al. (2018),
This study
A. pseudoglaucus
Blochwitz*
Aspergillaceae
E
China
Dissanayake et al. (2018)
A. ustus (Bainier) Thom
& Church
Aspergillaceae
U
Italy
Greuter et al. (1991)
Aspergillus sp.*
Aspergillaceae
P, E,
S
China, France, Italy,
Korea,South Africa, Spain,
Switzerland
Larignon and Dubos (2001),
Halleen et al. (2003), Casieri
et al. (2009), Gonzalez and
Tello (2011), Mondello
et al. (2013), Oh et al.
(2014), Dissanayake et al.
(2018), This study
Asperisporium
minutulum (Sacc.)
Deighton
Mycosphaerellaceae
E
USA
Schubert and Braun (2005)
A. vitiphyllum
(Speschnew) Deighton
Mycosphaerellaceae
E
China, Europe, Russia,
Uzbekistan
Elenkin (1909), Gaponenko
(1965), Sutton (1975),
Zhuang (2005)
Athelia rolfsii (Curzi)
C.C. Tu & Kimbr.
Atheliaceae
P, S
Mauritius, New Zealand,
Taiwan
Aureobasidium pullulans
(de Bary) G. Arnaud.*
Saccotheciaceae
E, S
Australia, China, France,
Germany, Greece, Italy,
South Africa, Spain, Poland,
USA
Orieux and Felix (1968),
Anonymous (1979),
Pennycook (1989)
Setati et al. (2015), Morgan
and Michailides (2004),
Mulenko et al. (2008),
Gonzalez and Tello (2011),
Sanoamuang et al. (2013),
Fischer et al. (2016),
Dissanayake et al. (2018),
This study, Jayawardena
et al. (2018)
Bunch rot,
canker, sour
rot
Sour rot
Aureobasidium sp.*
Saccotheciaceae
S
China
This study
Bactrodesmium pallidum
M.B. Ellis
Dothideomycetes
genera incertae
sedis
S
Russia
Melnik and Popushoi (1992)
Bartalinia robillardoides
Tassi
Sporocadaceae
S
India
Mathur (1979)
Beauveria bassiana
(Bals.-Criv.) Vuill*
Cordycipitaceae
P, E
Spain
Gonzalez and Tello (2011),
Garcia-Benavides et al.
(2013)
Bertia vitis Schulzer
Bertiaceae
S
Croatia, Portugal
Schulzer (1870), Unamuno
(1941)
Bionectria ochroleuca
(Schwein.) Schroers &
Samuels*
Bionectriaceae
S
Switzerland
Casieri et al. (2009)
Bipolaris maydis (Y.
Nisik. & C. Miyake)
Shoemaker*
Pleosporaceae
S
China
This study, Jayawardena et al.
(2018)
123
U
Fungal Diversity (2018) 90:1–84
19
Table 6 (continued)
Species
Family
Life
mode
B. sorokiniana (Sacc.)
Shoemaker*
Pleosporaceae
Biscogniauxia capnodes
(Berk.) Y.M. Ju & J.D.
Rogers
Disease caused
Locality
References
E
China
Dissanayake et al. (2018)
Boliniaceae
S
Taiwan
Ju and Rogers (1999)
B. mediterranea (De
Not.) Kuntze
Boeremia exigua var.
exigua (Desm.)
Aveskamp*
Boliniaceae
S
USA
Anonymous (1960)
Didymellaceae
P
Black spot
Italy
Balmas et al. (2005)
Botryodiplodia
palmarum (Cooke)
Petr. & Syd.
Botryosphaeriaceae
P
Canker
India
Mathur (1979)
B. vitis Sousa da Câmara
Botryosphaeriaceae
P
Canker
Pakistan, Portugal
Sousa da Câmara (1950),
Ahmad et al. (1997)
Botryodiplodia sp.
Botryosphaeriaceae
P
Canker
Argentina, Brazil
Mendes et al. (1998), Gatica
et al. (2001)
Botryosphaeria
bondarzewii L.
A. Kantsch.
Botryosphaeriaceae
S
Russia, USA
Kantschaveli (1928), Nagorny
(1930)
B. dothidea (Moug. ex
Fr.) Ces. & De Not.*
Botryosphaeriaceae
P, E,
S
Botryosphaeria
die back,
Macrophoma
rot
Argentina, Australia, Brazil,
Canda, Chile, China, France,
Germany, Iran, Italy, Japan,
South Africa, Portugal, Spain,
USA, New Zealand, Tunisia,
Turkey, Uruguay
Milholland (1994), Phillips
(1998, 2000), Slippers et al.
(2007a, b), Larignon and
Dubos (2001), Halleen et al.
(2003), van Niekerk et al.
(2006), Kobayashi (2007),
Luque et al. (2009), Pitt
et al. (2010), Qiu et al.
(2011), Úrbez-Torres
(2011), Úrbez-Torres et al.
(2012, 2013a, b), Abreo
et al. (2012), Arzanlou et al.
(2012), Baskarathevan et al.
(2012), Yan et al. (2012),
Akgul et al. (2014a), Chebil
et al. (2014), Carlucci et al.
(2015), Fischer et al. (2016),
Dissanayake et al. (2018),
This study, Jayawardena
et al. (2018)
B. vitis Niessl
Botryosphaeriaceae
P
Die back
Czech Republic
Niessl (1871)
Botryosphaeria sp.*
Botryosphaeriaceae
P, E
Botryosphaeria
die back,
Macrophoma
rot
Australia, China, Japan, South
Africa, Spain
Fourie and Halleen (2002),
Halleen et al. (2003),
Gimenez-Jaime et al.
(2006), Kobayashi (2007),
Martin and Cobos (2007),
Sosnowski et al. (2007),
Dissanayake et al. (2018)
Botrytis ampelophila
Speg.
Sclerotiniaceae
S
Argentina
Farr (1973)
B. californica S. Saito &
C.L. Xiao*
Sclerotiniaceae
P
California, USA
Saito et al. (2016)
Botrytis bunch
rot, Leaf
blight
123
20
Fungal Diversity (2018) 90:1–84
Table 6 (continued)
Species
Family
Life
mode
Disease caused
Locality
References
B. cinerea Pers.*
Sclerotiniaceae
P, E,
S
Botrytis bunch
rot, Leaf
blight
Australia, Brazil, Bulgaria,
Chile, China, France, Greece,
Germany, Hawai, Italy,
Korea, Libya, New Zealand,
Pakistan, Poland, Portugal,
Scotland, Spain, Switzerland,
USA, Zimbabwe
Foister (1961), Whiteside
(1966), El-Buni and Rattan
(1981), Raabe et al. (1981),
Lee et al. (1991), Mendes
et al. (1998), Holevas et al.
(2000), Phillips (2000),
Gadgil (2005), Mulenko
et al. (2008), Bobev (2009),
Casieri et al. (2009), Gao
et al. (2009), Gonzalez and
Tello (2011), Walker et al.
(2011), Fournier et al.
(2013), Piqueras et al.
(2014), Saito et al. (2016),
Dissanayake et al. (2018),
Javed et al. (2017), This
study, Jayawardena et al.
(2018)
B. pseudocinerea A.S.
Walker, A. Gautier*
Sclerotiniaceae
P
France, Germany, New
Zealand, USA
Walker et al. (2011), Saito
et al. (2016)
B. sinoviticola J. Zhang,
Y. J. Zhou & G. Q. Li*
Sclerotiniaceae
P
Botrytis bunch
rot, Leaf
blight
Botrytis bunch
rot, Leaf
blight
China
Zhou et al. (2014)
Botrytis sp.*
Sclerotiniaceae
P, E,
S
Chile, China, Italy, Japan,
Mexico, USA
Mujica and Vergara (1945),
Anonymous (1960), Alvarez
(1976), Kobayashi (2007),
Liu et al. (2016a),
Dissanayake et al. (2018),
Jayawardena et al. (2018)
Briosia ampelophaga
Cavara
Ascomycota genera
incertae sedis
P
Brown Zonate
Spot of
Grape/Leaf
blotch
Japan, Russia, USA
Greene (1955), Anonymous
(1960), Melnik and
Popushoi (1992), Nakagiri
et al. (1994), Kobayashi
(2007)
Cadophora fastigiata
Lagerb. & Melin*
Ploettnerulaceae
P, S
Wood pathogen
Germany, Switzerland,
Casieri et al. (2009), Fischer
et al. (2016)
C. luteo-olivacea (J.F.H.
Beyma) T.C. Harr. &
McNew*
Ploettnerulaceae
P
Wood pathogen
Germany, Japan, Switzerland,
Uruguay
Casieri et al. (2009), Abreo
et al. (2012), Fischer et al.
(2016), Nakaune et al.
(2016)
C. novi-eboraci R
Travadon, DP
Lawrence, S RooneyLatham, WD Gubler,
PE Rolshausen & K
Baumgartner*
Ploettnerulaceae
P
Wood pathogen
North America
Travadon et al. (2015)
C. orientoamericana R
Travadon, DP
Lawrence, S RooneyLatham, WD Gubler,
PE Rolshausen & K
Baumgartner*
Ploettnerulaceae
P
Wood pathogen
North America
Travadon et al. (2015)
C. spadicis R Travadon,
DP Lawrence, S
Rooney-Latham, WD
Gubler, PE Rolshausen
& K Baumgartner*
Ploettnerulaceae
P
Wood pathogen
North America
Travadon et al. (2015)
123
Fungal Diversity (2018) 90:1–84
21
Table 6 (continued)
Species
Family
Life
mode
Disease caused
Locality
References
C. viticola D. Gramaje,
L. Mostert &
Armengol*
Ploettnerulaceae
P, S
Wood pathogen
Spain
Crous et al. (2015)
Cadophora sp.*
Ploettnerulaceae
E, S
China
Dissanayake et al. (2018),
This study
Calonectria kyotensis
Terash.
C. macrospora Sacc. &
Speg.
Nectriaceae
P
New Zealand
Pennycook (1989)
Nectriaceae
P
Italy
Saccardo (1878), Farr (1973)
Calycella sarmentorum
(De Not.) Boud.
Helotiaceae
S
Italy, Portugal
Kuntze (1898), Unamuno
(1941)
Camarosporium
viniferum S. Ahmad
Camarosporiaceae
E
Central Asia, Pakistan
Ahmad (1969), Koshkelova
and Frolov (1973), Ahmad
et al. (1997)
C. viticola (Cooke &
Harkn.) Sacc.
Camarosporiaceae
E
USA
Saccardo (1878)
Camillea tinctor (Berk.)
Læssøe, J.D. Rogers &
Whalley
Graphostromataceae
S
USA
Hanlin (1963)
Campylocarpon
fasciculare Schroers,
Halleen & Crous*
Nectriaceae
P
Wood canker,
Black foot
disease
Brazil, Italy, South Africa,
Turkey
Halleen et al. (2003), Abreo
et al. (2010), Petit et al.
(2011), Correia et al. (2013),
Akgul et al. (2014b), ÚrbezTorres et al. (2014),
Carlucci et al. (2017),
Gonzalez and Chaverri
(2017)
C. pseudofasciculare
Halleen, Schroers &
Crous*
Nectriaceae
P
Black foot
Brazil, South Africa, Uruguay
Abreo et al. (2010, 2012),
Petit et al. (2011), Correia
et al. (2013), Úrbez-Torres
et al. (2014), Gonzalez and
Chaverri (2017)
Capnodium citri Berk. &
Desm.
Capnodiaceae
P
Bunch rot
Italy, Greece, Portugal, Spain
Pantidou (1973), Greuter et al.
(1991), Checa (2004)
Capnodium sp.
Capnodiaceae
P
Bunch rot
Brazil, Venezuela
Cephalosporium sp.
Hypocreales incertae
sedis
P
Black measles
Greece, Mexico, Greece, USA
Urtiaga (1986), Mendes et al.
(1998)
Chiarappa (1959), Pantidou
(1973), Alvarez (1976),
Holevas et al. (2000)
Ceratobasidium
cornigerum (Bourdot)
D.P. Rogers
Ceratobasidiaceae
E
Spain
Gonzalez and Tello (2011)
Ceratobasidium sp.*
Ceratobasidiaceae
E, S
China, Switzerland
Casieri et al. (2009), This
study
Cercospora coryneoides
Savul. & Rayss
Mycosphaerellaceae
P
Leaf spot
Palestine
Savulescu and Rayss (1935)
C. fuckelii (Thüm.) Jacz.
Mycosphaerellaceae
P
Leaf spot
Asia
Chupp (1953)
C. judaica Rayss
C. roesleri (Catt.) Sacc.*
Mycosphaerellaceae
Mycosphaerellaceae
P
P
Leaf spot
Leaf spot
Palestine
China, Cyprus, Egypt, France,
Scotland
Chupp (1953)
Chupp (1953), Georghiou and
Papadopoulos (1957),
Foister (1961), Tai (1979),
Soliman et al. (2016)
C. sessilis Sorokin
Mycosphaerellaceae
P
Leaf spot
Russia
Pollack (1987)
C. vitiphylla (Speschnew)
Barbarin
Mycosphaerellaceae
P
Leaf spot
Palestine
Savulescu and Rayss (1935)
Black foot
disease
Black foot
disease
123
22
Fungal Diversity (2018) 90:1–84
Table 6 (continued)
Species
Family
Life
mode
Disease caused
Locality
References
C. zebrina Pass.*
Mycosphaerellaceae
P
Leaf spot
Iran
Bakhshi et al. (2012)
Cercospora sp.
Mycosphaerellaceae
P
Leaf spot
Cuba, Hawaii, Mexico, USA
Denaree and Runner (1942),
Greene (1956), Raabe
(1966), Alvarez (1976),
Grand (1985), Urtiaga
(1986)
Chaetomium globosum
Kunze ex Fr.*
Chaetomiaceae
E, S
China, Italy, Spain,
Switzerland,
Casieri et al. (2009), Gonzalez
and Tello (2011),
Dissanayake et al. (2018),
This study, Jayawardena
et al. (2018)
C. nigricolor L.M.
Ames*
Chaetomiaceae
E
India, Switzerland
Pande (2008), Casieri et al.
(2009)
Chaetomium sp.*
Chaetomiaceae
E, S
Spain, Switzerland, China
Casieri et al. (2009), Gonzalez
and Tello (2011), This study
Chaetothyrium
javanicum (Zimm.)
Boedijn
Chaetothyriaceae
P
China, Taiwan
Tai (1979)
Chalastospora gossypii
(Jacz.) U. Braun &
Crous*
Cheilymenia
theleboloides (Alb. &
Schwein.) Boud.
Pleosporaceae
E
USA
Crous et al. (2009)
Pyronemataceae
S
Chile
Mujica and Vergara (1945)
Chrysosporium pilosum
Gené, Guarro & Ulfig*
Onygenaceae
S
China
This study
Chrysosporium sp.*
Cladochytrium viticola
Prunet
Onygenaceae
Cladochytriaceae
S
P
Wood
China
Algeria, Gaul, Tunisia, USA
This study
Saccardo (1878)
Cladosporium
aggregatocicatricatum
Bensch, Crous & U.
Braun*
Cladosporiaceae
P
Fruit rot
USA
Bensch et al. (2015)
C. ampelinum Pass.
Cladosporiaceae
P
Leaf spot
Austria, Germany, France,
Italy, Portugal
Passerini (1872)
C. asperulatum Bensch,
Crous & U. Braun
Cladosporiaceae
P
Fruit rot
USA
Bensch et al. (2015)
Sooty mold
C. autumnale Kübler
Cladosporiaceae
E
Switzerland
Dugan et al. (2004)
C. baccae Verwoerd &
Dippen.
Cladosporiaceae
P
Fruit rot
South Africa
Braun et al. (2003), Dugan
et al. (2004)
C. cladosporioides
(Fresen.) G.A. de
Vries*
Cladosporiaceae
P, E,
S
Fruit rot
Chile, China, Italy, Japan,
Switzerland, USA
Briceno and Latorre (2007),
Kobayashi (2007), Casieri
et al. (2009), Bensch et al.
(2015), Swett et al. (2016),
Dissanayake et al. (2018),
This study, Jayawardena
et al.(2018)
C. cucumerinum Ellis &
Arthur*
Cladosporiaceae
S
Italy
This study, Jayawardena
et al.(2018)
C. fasciculatum Corda
Cladosporiaceae
Russia, Spain, Uzbekistan
Gonzalez Fragoso (1921),
Nagorny (1930)
C. herbarum (Pers.) Link
Cladosporiaceae
Australia,Chile, Spain
Cook and Dubé (1989),
Briceno and Latorre (2007),
Gonzalez and Tello (2011)
123
P, E
Fruit rot
Fungal Diversity (2018) 90:1–84
23
Table 6 (continued)
Species
Family
Life
mode
Disease caused
Locality
References
C. limoniforme Bensch,
Crous & U. Braun*
Cladosporiaceae
P
Fruit rot
USA
Bensch et al. (2015), Swett
et al. (2016)
C. longipes Sorokin
Cladosporiaceae
E
Caucasus
Dugan et al. (2004)
C. macrocarpum Preuss
Cladosporiaceae
P
Fruit rot
China
Zhang (2003)
C. oxysporum Berk. &
M.A. Curtis
Cladosporiaceae
P
Fruit rot
India
Sarbhoy et al. (1971)
C. pestis Thüm
Cladosporiaceae
E
Austria
Dugan et al. (2004)
C. ramotenellum K.
Schub., Zalar, Crous &
U. Braun*
Cladosporiaceae
P
China, USA
Swett et al. (2016),
Dissanayake et al. (2018)
C. rectoides Bensch,
H.D. Shin, Crous & U.
Braun*
Cladosporiaceae
E
Korea
Bensch et al. (2015)
C. roesleri Catt.
Cladosporiaceae
E
Austria, France, Cyprus,
Pakistan
Georghiou and Papadopoulos
(1957), Ahmad (1969),
Ahmad et al. (1997)
C. silences Crous*
Cladosporiaceae
P
Fruit rot
China
Dissanayake et al. (2018)
C. sphaerospermum
Penz.*
Cladosporiaceae
P, S
Fruit rot
Switzerland
Casieri et al. (2009)
C. tenellum K. Schub.,
Zalar, Crous & U.
Braun*
Cladosporiaceae
P
Fruit rot
USA
Swett et al. (2016),
Dissanayake et al. (2018)
C. tenuissimum Cooke*
Cladosporiaceae
P, E
Fruit rot
China
Zhang (2003), Dissanayake
et al. (2018)
C. uvarum McAlpine
Cladosporiaceae
S
Australia, China
Zhang (2003), Dugan et al.
(2004)
C. viride (Fresen.) Z.Y.
Zhang & T. Zhang
Cladosporiaceae
P
Fruit rot
China
Dugan et al. (2004)
C. vitis-frutigeni Herb.
Cladosporiaceae
E
USA
Dugan et al. (2004)
Cladosporium sp.*
Cladosporiaceae
P, E,
S
Fruit rot
Chile, China, Italy, Korea,
USA, Venezuela
Mujica and Vergara (1945),
Anonymous (1960), Briceno
and Latorre (2008),
Mondello et al. (2013), Oh
et al. (2014), Dissanayake
et al. (2018), This study
Clathrospora
turkestanica
Domashova
Pleosporaceae
E
Central Asia
Koshkelova and Frolov (1973)
Claviceps sp.*
Clavicipitaceae
S
China
This study
Clonostachys rosea
(Link) Schroers,
Samuels, Seifert & W.
Gams*
Bionectriaceae
P, E,
S
Wood decay,
Root rot
China, Switzerland
Casieri et al. (2009), This
study, Jayawardena et al.
(2018)
Clonostachys sp.*
Bionectriaceae
P, E,
S
Wood decay,
Root rot
China, South Africa
Halleen et al. (2003), This
study
Cochliobolus geniculatus
R.R. Nelson
Pleosporaceae
P
Leaf spot
Brunei
Peregrine and Ahmad (1982)
Colletotrichum acutatum
J.H. Simmonds*
Glomerellaceae
P
Ripe rot
Australia, Japan, New Zealand,
USA
C. aenigma B.S. Weir &
P.R. Johnston*
Glomerellaceae
P
Ripe rot
China
Miller (1991), Kummuang
et al. (1996), Guerber et al.
(2003), Kobayashi (2007),
Shivas et al. (2016)
Yan et al. (2015)
C. ampelinum Cavara
Glomerellaceae
E
China, Italy
Cavara (1889), Tai (1979)
Fruit rot
123
24
Fungal Diversity (2018) 90:1–84
Table 6 (continued)
Species
Family
Life
mode
Disease caused
Locality
References
C. clidemia B.S. Weir &
P.R. Johnston*
Glomerellaceae
P
Ripe rot
USA
Weir et al. (2012)
C. dematium (Pers.)
Grove*
Glomerellaceae
E, S
Russia, South Africa
Damm et al. (2009), This
study, Jayawardena et al.
(2018)
C. fioriniae Marcelino &
Gouli ex R.G. Shivas &
Y.P. Tan*
Glomerellaceae
P
Ripe rot
Italy, Portugal
Faedda et al. (2011), Damm
et al. (2012)
C. fructicola Prihastuti,
L. Cai & K.D. Hyde*
Glomerellaceae
P
Ripe rot, Leaf
spot, Sunken
shoot and
stem canker
China
Peng et al. (2013)
C. gloeosporioides
(Penz.) Penz. & Sacc.*
Glomerellaceae
P
Ripe rot
Australia, Barbodos, Brazil,
Brunei, China, Cuba, India,
Japan, Korea, Mynmar, New
Zealnd, South Africa,
Taiwan, USA
Chandra (1974), Norse
(1974), Anonymous (1979),
Tai (1979), Peregrine and
Ahmad (1982), Urtiaga
(1986), Pennycook (1989),
Mendes et al. (1998), Cho
and Shin (2004), Lubbe
et al. (2004), Gadgil (2005),
Kobayashi (2007), Thaung
(2008c), Weir et al. (2012)
C. godetiae Neerg.*
Glomerellaceae
P, S
Ripe rot
Italy, UK
Baroncelli et al. (2014),
Zapparata et al. (2017), This
study, Jayawardena et al.
(2018)
C. hebeiense XH Li, Y
Wang, KD Hyde.
MMRS* Jayawardena,
JY Yan
Glomerellaceae
P
Twig
anthracnose,
Ripe rot
China
Yan et al. (2015), This study,
Jayawardena et al. (2018)
C. nymphaeae (Pass.)
Aa*
Glomerellaceae
P
Ripe rot
China
Liu et al. (2016b)
C. siamense Prihastuti, L.
Cai & K.D. Hyde*
Glomerellaceae
P, S
Ripe rot
Italy, USA
Weir et al. (2012), This study,
Jayawardena et al. (2018)
C. truncatum (Schwein.)
Andrus & W.D.
Moore*
Glomerellaceae
P
Ripe rot
China, India, Italy, Switzerland
Farr (1973), Casieri et al.
(2009), Sawant et al. (2012),
Pan et al. (2016), This study,
Jayawardena et al. (2018)
C. viniferum L.J. Peng, L.
Cai, K.D. Hyde & Zi Y.
Ying*
Glomerellaceae
P, S
Ripe rot
China
Peng et al. (2013), Yan et al.
(2015), This study,
Jayawardena et al. (2018)
Colletotrichum sp.
Glomerellaceae
P
Ripe rot, Wood
necrosis
Cuba, Mexico, Spain
Alvarez (1976), Arnold
(1986), Gonzalez and Tello
(2011)
Collophorina paarla
(Damm & Crous)
Damm & Crous*
Leotiomycetes genera
incertae sedis
P
Wood necrosis
Germany
Fischer et al. (2016)
C. rubra (Damm &
Crous) Damm &
Crous*
Leotiomycetes genera
incertae sedis
P
Wood necrosis
Spain
Garcia-Benavides et al. (2013)
Coniella castaneicola
(Ellis & Everh.) B.
Sutton
Schizoparmaceae
P
White rot
Japan, USA
Nag Raj (1993), Kobayashi
(2007)
123
Fungal Diversity (2018) 90:1–84
25
Table 6 (continued)
Species
Family
Life
mode
Disease caused
Locality
References
C. diplodiella (Speg.)
Petr. & Syd.*
Schizoparmaceae
P
White rot
Africa, Australia, Bulgaria,
China, France, Germany,
Greece, India, Italy, South
Africa
Sutton (1969), Pantidou
(1973), Mathur (1979),
Zhuang (2001), van Niekerk
et al. (2004b), Bobev
(2009), Chethana et al.
(2017)
C. diplodiopsis (Crous &
Van Niekerk) L.V.
Alvarez & Crous*
Schizoparmaceae
P
White rot
France, Germany, Italy, South
Africa, Switzerland
van Niekerk et al. (2004b),
Chethana et al. (2017)
C. fragariae (Oudem.) B.
Sutton
Schizoparmaceae
P
White rot
Germany, Japan
van Niekerk et al. (2004b),
Kobayashi (2007)
C. granati (Sacc.) Petr. &
Syd.*
Schizoparmaceae
P
White rot
Italy
van Niekerk et al. (2004b),
Chethana et al. (2017)
C. petrakii B. Sutton*
Schizoparmaceae
P, S
White rot
France, India
Nag Raj (1993), Chethana
et al. (2017)
C. vitis Chethana, Yan, Li
& K. D. Hyde*
Schizoparmaceae
P
White rot
China
Chethana et al. (2017), This
study, Jayawardena et al.
(2018)
Wood necrosis
Coniella sp.*
Schizoparmaceae
P
Coniocessia sp.*
Coniocessiaceae
S
India
Chethana et al. (2017)
China
This study
Coniochaeta hoffmannii
(J.F.H. Beyma) Z.U.
Khan, Gené & Guarro*
Coniochaetaceae
P
Germany, Switzerland
Casieri et al. (2009), Fischer
et al. (2016)
Coniolariella sp.*
Xylariaceae
Coniothecium viticola
Cooke & Massee
Helotiales incertae
sedis
S
China
This study
S
UK
Saccardo (1878)
Coniothyrium ampelinum
Cooke
Coniothyriaceae
E
USA
Cooke (1878)
C. berlandieri Viala &
Sauv.
Coniothyriaceae
P
Cambodia, USA
Anonymous (1960),
Litzenberger et al. (1962)
C. iranicum Esfand.
Coniothyriaceae
E
Central Asia
Koshkelova and Frolov (1973)
C. vitivorum Miura
Coniothyriaceae
E
Cophinforma mamane
(D.E. Gardner) A.J.L.
Phillips & A. Alves*
Botryosphaeriaceae
P
Coprinellus radians
(Desm.) Vilgalys,
Hopple & Jacq.
Johnson*
Psathyrellaceae
S
Corticium appalachiense
(Burds. & M.J. Larsen)
M.J. Larsen
Corticiaceae
P, S
C. centrifugum (Weinm.)
Fr.
Corticiaceae
P, S
Corticium sp.
Corticiaceae
S
Coryneopsis microsticta
(Berk. & Broome)
Grove
Discosiaceae
P
Corynespora cassiicola
(Berk. & M.A. Curtis)
C.T. Wei
Coryneum viticola Ellis
& Everh.
Corynesporascaceae
P
Pseudovalsaceae
S
Bunch rot
Leaf spot
China
Tai (1979)
Brazil
Correia et al. (2013)
Switzerland
Casieri et al. (2009)
Wood decay
USA
Burdsall (1976)
Wood decay
China
Tai (1979)
USA
Anonymous (1960)
Stem lesions
Poland, Portugal
de Sousa Dias and Lucas
(1972), Mulenko et al.
(2008)
Leaf spot
USA
Alfieri Jr. et al. (1984, 1994)
USA
Anonymous (1960)
Canker, Die
back
123
26
Fungal Diversity (2018) 90:1–84
Table 6 (continued)
Species
Family
Life
mode
Crepidotus viticola S.
Imai
Inocybaceae
Cryptocline cinerascens
(Bubák) Arx
Disease caused
Locality
References
S
Japan
Petrak (1953)
Ascomycota genera
incertae sedis
E
Japan
Kobayashi (2007)
Cryptococcus sp.*
Tremellaceae
E, S
China
Dissanayake et al. (2018),
This study
Cryptophaeella
trematosphaeriicola
Frolov
Montagnulaceae
E
Central Asia
Koshkelova and Frolov (1973)
Cryptosphaeria
pullmanensis Glawe*
Diatrypaceae
P
Canker
USA
Cryptosporella viticola
Shear
Valsaceae
P
Fruit rot, Dead
arm
China, Greece, Korea, USA
Trouillas and Gubler (2010),
Trouillas et al. (2010),
Úrbez-Torres et al. (2012)
Hewitt (1951), Tai (1979),
Holevas et al. (2000), Cho
and Shin (2004)
Cryptovalsa ampelina
Abbado*
Diatrypaceae
P
Eutypa dieback
Australia, Austria, Chile,
France, Hungary, Italy,
Portugal, South Africa, Spain,
USA
Unamuno (1941), Petrak
(1953), Mostert et al.
(2004), Lardner et al.
(2005), Sosnowski et al.
(2007), Luque et al. (2009),
Martin et al. (2009),
Trouillas and Gubler (2010),
Trouillas et al. (2010, 2011),
Diaz et al. (2011), White
et al. (2011), Úrbez-Torres
et al. (2012), Pitt et al.
(2013), Li et al. (2016designated reference
specimen), This study,
Jayawardena et al. (2018)
C. protracta (Pers.) De
Not.
Diatrypaceae
P
Eutypa dieback
Greece
Pantidou (1973)
C. rabenhorstii
(Nitschke) Sacc.*
Diatrypaceae
P
Eutypa dieback
Australia
Trouillas et al. (2011), Pitt
et al. (2013)
Eutypa dieback
Cryptovalsa sp.*
Diatrypaceae
P
Curvularia americana Da
Cunha, Madrid, Gené &
Cano*
Pleosporaceae
E
Curvularia sp.*
Pleosporaceae
E
Cylindrocarpon
destructans (Zinssm.)
Scholten*
Diatrypaceae
P, E
Black foot
C. lichenicola (C.
Massal.) D. Hawksw.
Diatrypaceae
P
C. ntricatea J.D.
MacDon. & E.E.
Butler*
Diatrypaceae
P
123
New Zealand
Lardner et al. (2005)
China
Dissanayake et al. (2018)
China
Dissanayake et al. (2018)
Argentina, Canada, France,
Iran, Italy, Portugal, Spain,
Tasmania, Uruguay
Gerlach and Ershad (1970),
Grasso (1984), Maluta and
Larignon (1991), Rego et al.
(2000), Gatica et al. (2001),
Seifert et al. (2003), Casieri
et al. (2009), Abreo et al.
(2010), Gonzalez and Tello
(2011)
Black foot
India
Booth (1966)
Black foot
Australia, Canada, France, Iran,
Portugal, Spain, Switzerland,
Uruguay, USA
Alaniz et al. (2007, 2009),
Petit and Gubler (2007),
Whitelaw-Weckert et al.
(2007), Casieri et al. (2009),
Luque et al. (2009), Abreo
et al. (2010, 2012), Petit
et al. (2011), Mohammadi
et al. (2013a)
Fungal Diversity (2018) 90:1–84
27
Table 6 (continued)
Species
Family
Life
mode
Disease caused
Locality
References
Cylindrocarpon sp.*
Diatrypaceae
P, S
Black foot
Canda, China, Lebanon,
Portugal, South Africa, Spain,
Switzerland, Tasmania, USA
Halleen et al. (2003),
Gimenez-Jaime et al.
(2006), Martin and Cobos
(2007), Whitelaw-Weckert
et al. (2007), Casieri et al.
(2009), Choueiri et al.
(2009), This study
Cylindrocladiella
lageniformis Crous,
M.J. Wingf. & Alfenas*
Nectriaceae
P
Black foot
South Africa, USA
Victor et al. (1998),
Boesewinkel (1982), Koike
et al. (2016)
C. parva (P.J. Anderson)
Boesew.*
Nectriaceae
P
Black foot
New Zealand, South Africa,
Spain
Van Coller et al. (2005),
Gadgil (2005), AgustiBrisach et al. (2012)
C. peruviana (Bat., J.L.
Bezerra & M.P.
Herrera) Boesew.*
Nectriaceae
P
Black foot
South Africa, USA
Boesewinkel (1982), Koike
et al. (2016)
C. pseudoparva L.
Lombard & Crous*
Nectriaceae
S
New Zealand
Boesewinkel (1982)
C. viticola Crous & Van
Coller*
Nectriaceae
P
Cutting rot of
grapevines,
Black foot
South Africa, USA
Hirooka et al. (2013)
C. vitis Crous &
Thangavel*
Nectriaceae
P
Black foot
New Zealand
Crous et al. (2017)
New Zealand
Boesewinkel (1982)
Pol2and
Mulenko et al. (2008)
Spain
Gonzalez and Tello (2011),
Garcia-Benavides et al.
(2013)
Cylindrocladiella sp.*
Nectriaceae
S
Cytospora ampelina
Sacc.
Valsaceae
P
C. chrysosperma (Pers.)
Fr.*
Valsaceae
E
Canker
C. cincta Sacc.*
Valsaceae
P
Canker
Iran
Fotouhifar et al. (2010)
C. leucostoma (Pers.)
Sacc.*
Valsaceae
P
Canker
Iran
Fotouhifar et al. (2010)
C. vinacea D.P. Lawr.,
Travadon & Pouzoulet*
Valsaceae
P
Canker
USA
Lawrence et al. (2017a)
C. viticola D.P. Lawr.,
Travadon & Pouzoulet*
Valsaceae
P
Canker
Canada, USA
Lawrence et al. (2017a)
C. vitis Mont.
Valsaceae
P
Canker
Central Asia, Greece, Portugal,
USA
Montagne (1856), Koshkelova
and Frolov (1973), Pantidou
(1973), Anonymous (1960),
Phillips (2000)
Dacrymyces viticola
Dacrymycetaceae
S
USA
Saccardo (1878)
Dactylellina sp.*
Orbiliaceae
S
China
This study
Dactylonectria
alcacerensis (A.
Cabral, Oliveira &
Crous)*
Nectriaceae
P
Black foot
Portugal, Spain
Agusti-Brisach et al. (2016),
Carlucci et al. (2017)
D. estremocensis (A.
Cabral, Nascimento &
Crous) L. Lombard &
Crous*
Nectriaceae
P
Black foot
Portugal
Agusti-Brisach et al. (2016),
Carlucci et al. (2017)
123
28
Fungal Diversity (2018) 90:1–84
Table 6 (continued)
Species
Family
Life
mode
Disease caused
Locality
References
D. macrodidyma
(Halleen, Schroers &
Crous)*
Nectriaceae
P, S
Black foot
Australia, Brazil, Canada, New
Zealand, Portugal, Slovenia,
South Africa, Switzerland,
USA
Casieri et al. (2009), Abreo
et al. (2010), Santos et al.
(2014), Úrbez-Torres et al.
(2014), Agusti-Brisach et al.
(2016), Carlucci et al.
(2017), This study
D. novozelandica (A.
Cabral & Crous) L.
Lombard & Crous*
Nectriaceae
P
Black foot
New Zealand, South Africa,
USA
Úrbez-Torres et al. (2014),
Carlucci et al. (2017)
D. pauciseptata
(Schroers & Crous) L.
Lombard & Crous*
Nectriaceae
P, S
Root rot, Black
foot
Brazil, Canada, New Zealand,
Portugal, Slovenia, Spain,
Uruguay
Abreo et al. (2010), AgustiBrisach et al. (2011), Martin
et al. (2011a), Petit et al.
(2011), Úrbez-Torres et al.
(2014), Santos et al. (2014)
D. pinicola L. Lombard
& Crous*
Nectriaceae
P
Black foot
Portugal
Carlucci et al. (2017),
D. torresensis (A. Cabral,
Rego & Crous) L.
Lombard & Crous*
Nectriaceae
P
Black foot
Australia, Canada, Italy, New
Zealand, Portugal, South
Africa, Spain, USA
Úrbez-Torres et al. (2014),
Agusti-Brisach et al. (2016),
Carlucci et al. (2017),
Gonzalez and Chaverri
(2017)
D. vitis (A. Cabral, Rego
& Crous) L. Lombard
& Crous*
Deconica horizontalis
(Bull.) Noordel.
Nectriaceae
P
Black foot
Portugal
Úrbez-Torres et al. (2014),
Carlucci et al. (2017)
Hymenogastraceae
S
South Africa
Doidge (1950)
Dendrophoma sp.
Chaetosphaeriaceae
S
Desarmillaria tabescens
(Scop.) R. A. Koch &
Aime
Devriesia sp.*
Physalacriaceae
P
Teratosphaeriaceae
Desmazierella sp.
Chorioactidaceae
Diaporthe ambigua
Nitschke*
Diaporthaceae
P
D. ampelina (Berkeley &
M.A. Curtis) R.R.
Gomes, C. Glienke &
Crous*
Diaporthaceae
D. mnivore (Delacr.)
Udayanga, P.W.Crous
& K.D.Hyde*
D. australafricana Crous
& Van Niekerk*
123
Japan
Kobayashi (2007)
Japan
Kobayashi (2007)
S
China
This study
S
Pakistan
Ahmad et al. (1997)
Canker
USA, South Africa
P, E,
S
Excoriose,
Dead arm,
Canker
Australia, Bulgaria, China,
France, India, Italy, Japan,
New Zealand, Poland, South
Africa, Spain, Switzerland,
Turkey, USA
van Niekerk et al. (2005),
White et al. (2011), ÚrbezTorres et al. (2013a, b),
Lawrence et al. (2015)
Phillips (2000), Zhuang
(2005), Kobayashi (2007),
Casieri et al. (2009),
Gonzalez and Tello (2011),
Garcia-Benavides et al.
(2013), Gomes et al. (2013),
Kepley et al. (2015),
Lawrence et al. (2015), Du
et al. (2016), This study,
Jayawardena et al. (2018)
Diaporthaceae
P
Canker
South Africa
van Niekerk et al. (2005),
Udayanga et al. (2011),
Gomes et al. (2013)
Diaporthaceae
P
Canker
Australia, South Africa, USA
van Niekerk et al. (2005),
Mostert et al. (2001),
Udayanga et al. (2012,
2014), Gomes et al. (2013),
Lawrence et al. (2015), Du
et al. (2016)
Root rot
Fungal Diversity (2018) 90:1–84
29
Table 6 (continued)
Species
Family
Life
mode
Disease caused
Locality
References
D. chamaeropis (Cooke)
R.R. Gomes, C.
Glienke & Crous
Diaporthaceae
P
Canker
USA
Lawrence et al. (2015)
D. eres Nitschke*
Diaporthaceae
P, S
Canker
Bulgaria, China, France,
Germany, Italy, Japan,
Switzerland, USA
Kobayashi (2007), Casieri
et al. (2009), Stoykov
(2012), Baumgartner et al.
(2013), Úrbez-Torres et al.
(2013a, b), Lawrence et al.
(2015), Cinelli et al. (2016),
Fischer et al. (2016), Bastide
et al. (2017), This study,
Jayawardena et al. (2018)
D. foenicula Niessl*
Diaporthaceae
P
Canker
South Africa, Portugal, USA
Luongo et al. (2011), ÚrbezTorres et al. (2013a, b),
Udayanga et al. (2014a, b),
Lawrence et al. (2015)
D. helianthi Munt.Cvetk., Mihaljc. & M.
Petrov*
Diaporthaceae
P
Canker
South Africa
van Niekerk et al. (2005),
Udayanga et al. (2011)
D. hongkongensis R.R.
Gomes, C. Glienke &
Crous*
Diaporthaceae
P
Canker
China
Dissanayake et al. (2015)
D. kyushuensis Kajitani
& Kanem.
D. longiparaphysata
(Uecker & K.C. Kuo)
Udayanga & Castl.*
Diaporthaceae
P
Canker
Japan
Diaporthaceae
P
Canker
Taiwan
Kanematsu et al. (2000),
Kobayashi (2007)
Uecker and Kuo (1992),
Udayanga et al. (2011)
D. nobilis Sacc. & Speg.*
Diaporthaceae
P
Canker
California
Lawrence et al. (2015)
D. novem M. Santos,
Vrandecic & A.J.L.
Phillips*
Diaporthaceae
P
Canker
California
Lawrence et al. (2015)
D. perjuncta Niessl
Diaporthaceae
P
Canker
Australia, Portugal, South
Africa
Phillips (1999), Mostert et al.
(2001)
D. perniciosa Marchal &
É.J. Marchal
Diaporthaceae
P
Canker
Bulgaria
Stoykow and Denchev (2006)
D. phaseolorum (Cooke
& Ellis) Sacc.*
Diaporthaceae
P
Canker
China, Switzerland
Casieri et al. (2009),
Dissanayake et al. (2015)
D. rudis (Fr.) Nitschke*
Diaporthaceae
P, S
Canker
Australia, Germany, Italy,
Portugal
Scheper et al. (2000), ÚrbezTorres et al. (2012), Gomes
et al. (2013), Udayanga et al.
(2014a, b), Huang et al.
(2015), This study,
Jayawardena et al. (2018)
D. sojae Lehman*
Diaporthaceae
P
Canker
China
Dissanayake et al. (2015)
D. vitimegaspora (K.C.
Kuo & L.S. Leu)
Rossman & Udayanga*
Diaporthaceae
P
Canker
Japan, Thailand, Thaiwan
Kuo and Leu (1998), van
Niekerk et al. (2005),
Udayanga et al. (2011)
Diaporthe sp.*
Diaporthaceae
P
Canker
Bulgaria, France, Italy, Japan,
Portugal, South Africa, Spain
Switzerland, USA
Kanematsu et al. (2000),
Mostert et al. (2001), van
Niekerk et al. (2005), Bobev
(2009), Casieri et al. (2009),
Santos et al. (2010), Luongo
et al. (2011), Úrbez-Torres
et al. (2013a, b)
123
30
Fungal Diversity (2018) 90:1–84
Table 6 (continued)
Species
Family
Life
mode
Disease caused
Locality
References
Diatrype nigerrima Ellis
& Everh.
Diatrypaceae
P
Eutypa dieback
USA
Ellis and Everhart (1904),
Cash (1952)
D. oregonensis Wehm.)
Rappaz*
Diatrypaceae
P
Eutypa dieback
USA
Trouillas and Gubler (2010),
Trouillas et al. (2010),
Úrbez-Torres et al.
(2013a, b)
D. stigma (Hoffm.) Fr.*
Diatrypaceae
P
Eutypa dieback
Spain, USA
Unamuno (1941), Trouillas
et al. (2010), Úrbez-Torres
et al. (2013a, b)
D. utahensis Rehm
Diatrypaceae
P
Eutypa dieback
India
Pande (2008)
D. whitmanensis J.D.
Rogers & Glawe*
Diatrypaceae
P
Eutypa dieback
USA
Trouillas and Gubler (2010),
Trouillas et al. (2010),
Úrbez-Torres et al.
(2013a, b)
Diatrype sp.*
Diatrypaceae
P
Eutypa dieback
Australia, USA
Trouillas et al. (2010, 2011),
Pitt et al. (2013), ÚrbezTorres et al.
(2012, 2013a, b)
Diatrypella
verrucaeformis (Ehrh.)
Nitschke*
D. vitis Ellis & Everh.
Diatrypaceae
P
Eutypa dieback
USA
Trouillas and Gubler (2010),
Trouillas et al. (2010)
Diatrypaceae
P
Eutypa dieback
China, USA
Cash (1952), Teng (1996)
D. vulgaris Trouillas,
W.M. Pitt & Gubler*
Diatrypaceae
P
Eutypa dieback
Australia
Trouillas et al. (2011), Pitt
et al. (2013)
Diatrypella sp.*
Diatrypaceae
P
Eutypa dieback
USA
Dictyosporium elegans
Corda
Dictyosporiaceae
P
Canker
Portugal
Trouillas and Gubler (2010),
Trouillas et al. (2010),
Úrbez-Torres et al. (2012)
de Sousa Dias et al. (1987)
D. toruloides (Corda)
Guég.
Dictyosporiaceae
P
Canker
Russia
Melnik and Popushoi (1992)
Didymella glomerata
(Corda) Q. Chen & L.
Cai*
Didymellaceae
E
Spain, Switzerland
Casieri et al. (2009), Gonzalez
and Tello (2011)
D. negriana (Thümen) Q.
Chen & L. Cai*
Didymellaceae
P, S
Germany, Italy
Chen et al. (2015), This study,
Jayawardena et al. (2018)
D. pomorum (Thümen)
Q. Chen & L. Cai*
Didymellaceae
S
Australia,China
Cook and Dubé (1989), This
study, Jayawardena et al.
(2018)
Didymosphaeria
bacchans Pass.
Didymosphaeriaceae
S
Italy
Greuter et al. (1991)
D. sarmenti (Cooke &
Harkn.) Berl. &
Voglino
Didymosphaeriaceae
P
Japan, Portugal, USA
Unamuno (1941), French
(1989), Kobayashi (2007)
Dinemasporium
pleurospora (Sacc.)
Shkarupa
Chaetosphaeriaceae
S
Pakistan, Poland
Ahmad (1969), Ahmad et al.
(1997), Mulenko et al.
(2008)
Diplodia ampelina Cooke
Botryosphaeriaceae
P
Portugal, USA
Cooke (1878), Saccardo and
Traverso (1903)
123
Black rot,
Canker
Shoot lesions
Canker
Fungal Diversity (2018) 90:1–84
31
Table 6 (continued)
Species
Family
Life
mode
Disease caused
Locality
References
D. bacchii Pass. & Thüm
Botryosphaeriaceae
P, S
Canker
Belgium, Italy, Portugal
Cooke (1878)
D. corticola A.J.L.
Phillips, A. Alves & J.
Luque*
Botryosphaeriaceae
P
Canker
Italy, Mexico, Spain, USA
Carlucci and Frisullo (2009),
Úrbez-Torres et al.
(2010a, b, c), Pintos et al.
(2011), Úrbez-Torres
(2011), Carlucci et al.
(2015)
D. intermedia A.J.L.
Phillips, J. Lopes & A.
Alves*
Botryosphaeriaceae
P
Canker
France
Comont et al. (2016)
D. mutila (Fr.) Mont.*
Botryosphaeriaceae
P, E
Canker
Australia, Canada, France,
Hungary, Italy, New Zealand,
Portugal, Spain, USA
Phillips (1998, 2000), Taylor
et al. (2005), Úrbez-Torres
et al. (2006), van Niekerk
et al. (2006), Martin and
Cobos (2007),
Baskarathevan et al.
(2008, 2012), Pitt et al.
(2010), Gonzalez and Tello
(2011), Qiu et al. (2011),
Úrbez-Torres (2011),
Whitelaw-Weckert et al.
(2013), Alves et al. (2014),
Carlucci et al. (2015)
D. nematospora Sacc.
Botryosphaeriaceae
S
Eritrea
Castellani and Ciferri (1937)
D. seriata (Fr.) Mont.*
Botryosphaeriaceae
P, E,
S
Canker
Australia, Bulgaria, Canada,
Chile, China, France,
Germany, Greece, Iran, Italy,
Lebanon, New Zealand,
Portugal, South Africa, Spain,
Switzerland, Tunisia
Uruguay, USA
Pantidou (1973), CastilloPando et al. (2001),
Larignon and Dubos (2001),
Halleen et al. (2003), Auger
et al. (2004a), Choueiri et al.
(2006), van Niekerk et al.
(2006), Slippers et al.
(2007a, b), Baskarathevan
et al. (2008), Epstein (2008),
Casieri et al. (2009), Luque
et al. (2009), Úrbez-Torres
(2011), Yan et al. (2011a, b),
Abreo et al. (2012), GarciaBenavides et al. (2013),
Mohammadi et al. (2013b),
Mondello et al. (2013),
Chebil et al. (2014), Fischer
et al. (2016), This study,
Jayawardena et al. (2018)
Diplodia sp.*
Botryosphaeriaceae
P
Canker
Belgium, Bulgaria, Cuba,
Mexico, South Africa
Diplodina vitis Brunaud
Gnomoniaceae
P
Root stock
disease
Central Asia
Greuter et al. (1991), van
Niekerk et al. (2004a),
Bobev (2009), Casieri et al.
(2009)
Koshkelova and Frolov (1973)
Discohainesia
oenotherae (Cooke &
Ellis) Nannf.
Dermateaceae
P
Leaf spot
USA
Anonymous (1960)
123
32
Fungal Diversity (2018) 90:1–84
Table 6 (continued)
Species
Family
Life
mode
Disease caused
Locality
References
Discosia artocreas
(Todd) Fr.
Sporocadaceae
P
Leaf spot
USA
Gilman (1932), Maneval
(1937), Cooke (1983)
D. vitis Schulzer
Sporocadaceae
P
Leaf spot
Hungary
Nag Raj (1993)
Discostroma corticola
(Fuckel) Brockmann
Sporocadaceae
P
Cane blight
New Zealand
Pennycook (1989)
Doratomyces stemonitis
(Pers.) F.J. Morton &
G. Sm.
Microascaceae
S
Argentina, Russia
Melnik and Popushoi (1992),
Carmaran and Novas (2003)
Dothiorella americana
Úrbez-Torres, Peduto &
Gubler*
Botryosphaeriaceae
P
Die back,
Canker
USA
Úrbez-Torres (2011), ÚrbezTorres et al. (2012)
D. iberica A.J.L. Phillips,
J. Luque & A. Alves*
Botryosphaeriaceae
P, S
Die back,
Canker
Australia, Italy, New Zealand,
Spain, USA
Úrbez-Torres et al. (2007),
Baskarathevan et al.
(2008, 2012), Úrbez-Torres
and Gubler (2009), Qiu et al.
(2011), Úrbez-Torres
(2011), Pitt et al. (2010),
McDonald and Eskalen
(2011), Carlucci et al.
(2015), Martin and Cobos
(2007), This study,
Jayawardena et al. (2018)
D. neclivora W.M. Pitt &
J.R. Úrbez-Torres*
Botryosphaeriaceae
P
Die back,
Canker
Australia
Pitt et al. (2015)
D. mnivore B.
T. Linaldeddu, A.
Deidda & B. Scanu*
Botryosphaeriaceae
P
Die back,
Canker
Australia
Linaldeddu et al. (2016)
D. reinformis (Viala &
Ravaz) Petr. & Syd
Botryosphaeriaceae
P, S
Die back,
Canker
Italy, Portugal, South Africa
D. sarmentorum (Fr.)
A.J.L. Phillips, Alves &
Luque*
Botryosphaeriaceae
P, S
Die back,
Canker
China, Italy, New Zealand,
Spain
Petrak and Sydow (1927),
Doidge (1950), Costa and
Camara (1952)
Martin and Cobos (2007),
Baskarathevan et al. (2012),
Carlucci et al. (2015), This
study, Jayawardena et al.
(2018)
D. vidmadera W.M. Pitt,
J.R. Úrbez-Torres,
Trouillas*
Botryosphaeriaceae
P
Die back,
Canker
Australia
Pitt et al. (2013), Linaldeddu
et al. (2016), Lawrence et al.
(2017b)
D. vinea-gemmae W.M.
Pitt & J.R. ÚrbezTorres*
Botryosphaeriaceae
P
Die back,
Canker
Australia
Pitt et al. (2015)
D. viticola A.J.L. Phillips
& J. Luque
Botryosphaeriaceae
P, S
Die back,
Canker
Spain
Luque et al. (2005)
Dothiorella sp.*
Botryosphaeriaceae
P
Die back,
Canker
Australia, Mexico, USA
Úrbez-Torres et al.
(2010a, b, c), Pitt et al.
(2015), Lawrence et al.
(2017b)
123
Fungal Diversity (2018) 90:1–84
33
Table 6 (continued)
Species
Family
Life
mode
Disease caused
Locality
References
Elsinoe ampelina Shear
Elsinoaeceae
P
Grape
antracnose
Barbados, Brazil, Bulgaria,
Cambodia,Chile,China,Cuba,
Haiti, Hong Kong, India,
Italy, Jamaica, Kenya,
Mauritius, Mexico, Myanmar,
New Zealand, Poland, South
Africa, Spain, Tanzania,
Trinidad and Tobago,
Thailand, USA, Venezuela,
Zimbabwe
Gilman and Archer (1929),
Jenkins and Bitancourt
(Jenkins and Bitancourt
1940–1963), Mujica and
Vergara (1945), Baker and
Dale (1951), Riley (1960),
Nattrass (1961),
Litzenberger et al. (1962),
Whiteside (1966), Orieux
and Felix (1968), Benjamin
and Slot (1969), Dennis
(1970), Norse (1974),
Alvarez (1976), Tai (1979),
Alfieri Jr. et al. (1984),
Grand (1985), Arnold
(1986), Pennycook (1989),
Greuter et al. (1991),
Mendes et al. (1998), Lu
et al. (2000), Zhuang (2001),
Mulenko et al. (2008),
Thaung (2008a, b, c), Bobev
(2009)
Emericella sp.*
Aspergillaceae
S
China
This study
Endobasidium
clandestinum
Speschnew
Exobasidiaceae
P
Root rot
Uzbekistan
Gaponenko (1965)
Endoconidioma populi
Tsuneda, Hambl. &
Currah*
Dothideaceae
P
Necrotic twigs
Iran
Mirzaei et al. (2015)
Epicoccum granulatum
Penz.
Didymellaceae
S
USA
Shaw (1973)
E. nigrum Link*
Didymellaceae
E, S
China, Italy, Spain, Switzerland
E. plurivorum (P.R.
Johnston) Q. Chen & L.
Cai
Didymellaceae
S
New Zealand
Phillips (2000), Casieri et al.
(2009), Gonzalez and Tello
(2011), This study,
Jayawardena et al. (2018)
Gadgil (2005)
Epicoccum sp.
Didymellaceae
S
France
Larignon and Dubos (1997),
Halleen et al. (2003)
Eriocercosporella vitisheterophyllae (Henn.)
U. Braun
Ascomycota genera
incertae sedis
P
Japan
Chupp (1953), Watson (1971)
Eriosphaeria oenotria
Sacc. & Speg.
Trichosphaeriaceae
S
Italy
Farr (1973)
Erysiphe necator
Schwein.
Erysiphaceae
P
Powdery
mildew
Australia, Belgium, Bulgaria,
Czechoslovakia, Denmark,
Finland, France, Germany,
Greece, Hungary, India,
Ishrael, Italy, Japan, Korea,
Netherlands, Peru, Poland,
Romania, Russia, Spain,
Sweden, Switzerland, Turkey,
UK, Yugoslavia
Greuter et al. (1991), Nomura
et al. (2003), Bolay (2005),
Ruszkiewicz-Michalska and
Michalski (2005), Amrani
and Corio-Costet (2006),
Paul and Thakur (2006),
Rusanov and Bulgakov
(2008), Voytyuk et al.
(2009), Park et al. (2010),
Bendezu-Euribe and
Alvarez (2012)
E. tuckeri Berk.
Erysiphaceae
P
Powdery
mildew
Spain
Unamuno (1941)
Leaf spot
123
34
Fungal Diversity (2018) 90:1–84
Table 6 (continued)
Species
Family
Life
mode
Disease caused
Locality
References
Erythricium salmonicolor
(Berk. & Broome)
Burds.
Corticiaceae
P
Sour rot
Thailand
Giatgong (1980)
Eucasphaeria capensis
Crous*
Niessliaceae
P
Eutypa dieback
Germany
Fischer et al. (2016)
Eutypa lata (Pers.) Tul.
& C. Tul.*
Diatrypaceae
P
Eutypa dieback
Australia, Brazil, Bulgaria,
Europe, France, Germany,
Greece, Italy, New Zealand,
Serbia, South Africa, Spain,
Switzerland, USA
Moller et al. (1974),
Pennycook (1989), Shivas
(1989), Carter (1991),
Larignon and Dubos (1997),
Mendes et al. (1998), Péros
et al. (1999), Holevas et al.
(2000), Rolshausen et al.
(2004, 2014), Lardner et al.
(2005), Sosnowski et al.
(2007), Bobev (2009),
Luque et al. (2009),
Trouillas et al. (2010, 2011),
White et al. (2011), ÚrbezTorres et al. (2012),
Živkovic et al. (2012),
Garcia-Benavides et al.
(2013), Travadon and
Baumgartner (2015),
Mayorquin et al. (2016)
E. laevata (Nitschke)
Sacc.*
Diatrypaceae
P
Eutypa dieback
Canada, USA
Rappaz (1987), Rolshausen
et al. (2004, 2014)
E. ludibunda Sacc.
E. leptoplaca (Durieu &
Mont.) Rappaz*
Diatrypaceae
Diatrypaceae
P
P
Eutypa dieback
Eutypa dieback
USA
Spain, South Africa, USA
Tiffany and Gilman (1965)
Luque et al. (2009), Trouillas
and Gubler (2004, 2010),
Úrbez-Torres et al. (2012)
Eutypa sp.*
Diatrypaceae
P
Eutypa dieback
Bulgaria, USA
Bobev (2009), Rolshausen
et al. (2014)
Eutypella aequilinearis
(Schwein.) Starbäck
Diatrypaceae
P
Eutypa dieback
Japan, USA
Rappaz (1987), Kobayashi
(2007)
E. aulacostroma (Kunze)
Berl.
Diatrypaceae
P
Eutypa dieback
Taiwan
Rappaz (1987)
E. citricola Speg.*
Diatrypaceae
P
Eutypa dieback
Australia, USA
Trouillas et al. (2011), Pitt
et al. (2013), Mayorquin
et al. (2016)
E. fraxinicola (Cooke &
Peck) Sacc.
Diatrypaceae
P
Eutypa dieback
USA
Hanlin (1963)
E. leprosa (Pers.) Berl.
Diatrypaceae
P
Eutypa dieback
Chile, Spain, Switzerland, USA
Rappaz (1987), Diaz et al.
(2011)
E. microtheca Trouillas,
W.M. Pitt & Gubler*
Diatrypaceae
P
Eutypa dieback
Australia, Mexico, USA
Trouillas et al. (2011), Pitt
et al. (2013), PaolinelliAlfonso et al. (2016),
Mayorquin et al. (2016)
E. vitis (Schwein.) Ellis
& Everh.*
Diatrypaceae
P
Eutypa dieback
Italy, Pakistan, South Africa,
Spain, Uruguay, USA
Greuter et al. (1991), Ahmad
et al. (1997), Luque et al.
(2009), White et al. (2011),
Úrbez-Torres et al. (2012),
Abreo et al. (2012),
Mayorquin et al. (2016)
Eutypella sp.*
Diatrypaceae
P
Eutypa dieback
USA
Trouillas et al. (2010), ÚrbezTorres et al. (2012),
Mayorquin et al. (2016)
123
Fungal Diversity (2018) 90:1–84
35
Table 6 (continued)
Species
Family
Life
mode
Disease caused
Locality
References
Excipula viticola
Schwein
Dermateaceae
P
On leaves
USA
Saccardo (1878)
Exosporium sultanae du
Plessis
Ascomycota genera
incertae sedis
S
South Africa
Gorter (1977)
Exophiala sp.*
Herpotrichiellaceae
E
China
Dissanayake et al. (2018)
Exserohilum rostratum
(Drechsler) K.J.
Leonard & Suggs*
Pleosporaceae
S
China
This study, Jayawardena et al.
(2018)
Floricola viticola
(Phukhamsakda,
Camporesi & K.D.
Hyde) Jaklitsch &
Voglmayr*
Teichosporaceae
S
Italy
Ariyawansa et al. (2015), This
study, Jayawardena et al.
(2018)
Fomes fomentarius (L.)
Fr.
Polyporaceae
P
Esca
China
Tai (1979)
F. igniarius (L.) Fr.*
Polyporaceae
P
Esca
France, USA
Chiarappa (1959), Cloete
et al. (2015)
Fomitiporia australiensis
M. Fisch., J. Edwards,
Cunningt. & Pascoe*
Hymenochaetaceae
P
Esca
Australia
Fischer et al. (2005), Cloete
et al. (2015)
F. capensis M. Fisch., M.
Cloete, L. Mostert, F.
Halleen*
Hymenochaetaceae
P
Esca
South Africa
Cloete et al. (2014)
F. mediterranea M.
Fisch.*
Hymenochaetaceae
P
Esca
Europe, Germany, Iran, Italy,
Spain, Turkey
Fischer et al. (2005), Martin
and Cobos (2007), Luque
et al. (2009), Mohammadi
and Banihashemi (2012),
Garcia-Benavides et al.
(2013), Mondello et al.
(2013), Akgul et al. (2015),
Cloete et al. (2015)
F. polymorpha M.
Fisch.*
Hymenochaetaceae
P
Esca
USA
Cloete et al. (2015)
F. punctata (P. Karst.)
Murrill*
Hymenochaetaceae
P
Esca
Australia, France, Iran, Italy
Larignon and Dubos (1997),
Pascoe and Cottral (2000),
Karimi et al. (2001), Cloete
et al. (2015)
Fomitiporia sp.*
Hymenochaetaceae
P
Esca
Italy, South Africa
White et al. (2011), Mondello
et al. (2013)
Fusarium acuminatum
Ellis & Everh.*
Nectriaceae
P
Wilt
Spain
Garcia-Benavides et al. (2013)
F. anthophilum (A.
Braun) Wollenw.
Nectriaceae
P
Wilt
Brazil
Mendes et al. (1998)
F. avenaceum (Fr.) Sacc.
Nectriaceae
P
Wilt
China, Italy
Tai (1979), Greuter et al.
(1991)
F. equiseti (Corda) Sacc.
Nectriaceae
P
Wilt
Brazil
Mendes et al. (1998)
F. fujikuroi Nirenberg
Nectriaceae
P
Wilt
Brazil
Mendes et al. (1998)
F. oxysporum Schltdl.*
Nectriaceae
P, E,
S
Wilt
Australia, Brazil, China, South
Africa, Spain
Gorter (1977), Mendes et al.
(1998), Castillo-Pando et al.
(2001), Gonzalez and Tello
(2011), This study,
Jayawardena et al. (2018)
F. poae (Peck) Wollenw.
Nectriaceae
P
Wilt
USA
Shaw (1973)
F. proliferatum
(Matsush.) Nirenberg*
Nectriaceae
P, E
Wilt
China, Spain
Gonzalez and Tello (2011),
Wang et al. (2015)
123
36
Fungal Diversity (2018) 90:1–84
Table 6 (continued)
Species
Family
Life
mode
Disease caused
Locality
References
F. schweinitzii Ellis &
Harkn.
Nectriaceae
P, E
Wilt
USA
Sumstine (1949), Cash (1952)
F. solani (Mart.) Sacc.*
Nectriaceae
P
Wilt
Brazil, India, Switzerland
Sarbhoy and Agarwal (1990),
Mendes et al. (1998), Casieri
et al. (2009)
F. viticola Thüm.
Nectriaceae
S
USA
Saccardo (1878)
F. volutella Ellis &
Everh.
Nectriaceae
P
Wilt
USA
Cash (1952)
Fusarium sp.*
Nectriaceae
P, S
Wilt
Australia, China, Germany,
Italy, South Africa,
Switzerland, Spain, Uruguay
Cook and Dubé (1989),
O’Donnell et al. (1998),
Halleen et al. (2003), Casieri
et al. (2009), Luque et al.
(2009), Abreo et al. (2010),
Mondello et al. (2013), This
study, Jayawardena et al.
(2018)
Fusicladium viticis M.B.
Ellis
Sympoventuriaceae
P
Leaf spot
China
Zhang (2003)
Geomyces pannorum
(Link) Sigler & J.W.
Carmich.*
Geomyces sp.
Myxotrichaceae
E
Switzerland
Casieri et al. (2009)
Myxotrichaceae
S
China
This study
Geotrichum candidum
Link
Dipodascaceae
E
Japan
Kobayashi (2007)
Geotrichum sp.
Dipodascaceae
E
Spain
Gonzalez and Tello (2011)
Gloniopsis praelonga
(Schwein.) Underw. &
Earle
Hysteriaceae
S
Germany
Lotz-Winter et al. (2011)
Glonium lineare (Fr.) De
Not.
Gloniaceae
S
Rhode Island
Goos (2010)
G. macrosporium Tracy
& Earle
Gloniaceae
S
USA
Parris (1959)
Glonium sp.
Gloniaceae
S
USA
Hanlin (1963)
Golovinomyces
biocellatus (Ehrenb.)
V.P. Heluta
Erysiphaceae
P
India
Paul and Thakur (2006)
Gonatobotrys flava
Bonord.
Ceratostomataceae
E
Poland
Mulenko et al. (2008)
Gonatobotryum sp.
Ascomycota genera
incertae sedis
E
Spain
Gonzalez and Tello (2011)
Graphium cinerellum
Speg.
Graphiaceae
P
Leaf spot
Italy
Farr (1973)
Greeneria uvicola (Berk.
& M.A. Curtis)
Punith.*
Diaporthales genera
incertae sedis
P
Bitter rot
Australia, Bulgaria, Brazil,
Cuba, India, Poland, South
Africa, Taiwan, Thailand,
Ukraine, Uruguay, USA
Cooke (1878), Simmonds
(1966), Gorter (1977),
Mathur (1979), Giatgong
(1980), Reddy and Reddy
(1983), Arnold (1986),
Kummuang et al. (1996),
Mendes et al. (1998),
Castillo-Pando et al. (2001),
Farr et al. (2001), Dudka
et al. (2004), Longland and
Sutton (2008), Mulenko
et al. (2008), Bobev (2009),
Navarrete et al. (2009),
Abreo et al. (2012)
123
Powdery
mildew
Fungal Diversity (2018) 90:1–84
37
Table 6 (continued)
Species
Family
Life
mode
Disease caused
Locality
References
Grovesinia moricola (I.
Hino) Redhead
Sclerotiniaceae
P
Bunch rot
USA
Grand (1985)
G. pyramidalis M.N.
Cline, J.L. Crane &
S.D. Cline
Sclerotiniaceae
P
Bunch rot
Japan
Kobayashi (2007)
Gymnascella sp.*
Gymnoascaceae
S
China
This study
Gyrothrix podosperma
(Corda) Rabenh.
Ascomycota genera
incertae sedis
S
Pakistan
Ahmad et al. (1997)
Hansfordia pulvinata
(Berk. & M.A. Curtis)
S. Hughes
Ascomycota genera
incertae sedis
S
Pakistan
Ahmad et al. (1997)
H. tonduzii (Speg.) Bat.
& A.F. Vital
Ascomycota genera
incertae sedis
S
Costa Rica
Batista and Ciferri (1962)
Hansfordia sp.*
Ascomycota genera
incertae sedis
S
China
This study
Hapalopilus rutilans
(Pers.) Murrill
Polyporaceae
S
USA
Gilbertson et al. (1974)
Helicobasidium mompa
Nobuj. Tanaka
Helicobasidiaceae
P
Root rot
Japan
Kobayashi (2007)
Helminthosporium
decacuminatum Thüm.
& Pass.
Dothideomycetes
genera incertae
sedis
P
Leaf spot
Greece, Macedonia
Konstantinia-Sulidu (1939),
Pantidou (1973)
H. siliquosum Berk. &
M.A. Curtis
Dothideomycetes
genera incertae
sedis
P
Twigs and leaf
spot
USA
Anonymous (1960)
H. velutinum (Link) Link
Dothideomycetes
genera incertae
sedis
S
Japan
Shirouzu and Harada (2004)
Helminthosporium sp.
Dothideomycetes
genera incertae
sedis
P
USA
Anonymous (1960), Alfieri Jr.
et al. (1984)
Hendersonia cookeana
Speg.
Ascomycota genera
incertae sedis
S
Italy
Spegazzini (1878), Farr
(1973)
H. corticalis Ellis &
Everh.
Ascomycota genera
incertae sedis
S
USA
Cash (1953)
H. sarmentorum
Westend.
Ascomycota genera
incertae sedis
P
Central Asia, Greece, Italy,
Pakistan, Spain, USA
Gonzalez Fragoso (1916),
Anonymous (1960), Ahmad
(1969), Koshkelova and
Frolov (1973), Pantidou
(1973), Greuter et al. (1991),
Ahmad et al. (1997)
H. tenuipes McAlpine
Ascomycota genera
incertae sedis
S
Greece
Pantidou (1973)
H. viticola S. Ahmad
Ascomycota genera
incertae sedis
S
Greece, Pakistan
Ahmad (1969), Pantidou
(1973), Ahmad et al. (1997)
Leaf spot
Twig lesions
Herpotrichia sp.
Melanommataceae
E
USA
Hanlin (1963)
Hormonema viticola F.
Laich & Stchigel*
Dothioraceae
E
Malaysia, Spain
Crous et al. (2015)
Humicola sp*.
Chaetomiaceae
E, S
China, Spain
Gonzalez and Tello (2011),
This study
Hydnum viticola
Hydnum sp.*
Hydnaceae
Hydnaceae
S
S
USA
China
Saccardo (1878)
This study
Hyaloceras viticola
(Cavara) Died.
Sporocadaceae
P
Italy
Saccardo (1878)
Fruits
123
38
Fungal Diversity (2018) 90:1–84
Table 6 (continued)
Species
Family
Life
mode
Hymenochaetopsis
intricata (Lloyd) S.H.
He & Jiao Yang
Hymenochaetaceae
S
Hypocrella reineckeana
Henn.
Clavicipitaceae
P
Hypoderma commune
(Fr.) Duby
H. rubi (Pers.) DC.
Rhytismataceae
Disease caused
Locality
References
Japan
Kobayashi (2007)
Niue
Dingley et al. (1981)
S
Portugal
Unamuno (1941)
Leaf spot
Rhytismataceae
S
China
Ying-Ren (2012)
Hypoxylon hypophlaeum
(Berk. & Ravenel) J.H.
Mill.
Hypoxylaceae
S
USA
Hanlin (1963)
H. lateripigmentum J.
Fourn., Kuhnert & M.
Stadler*
Hypoxylaceae
E
China
Dissanayake et al. (2018)
H. rubiginosum (Pers.)
Fr.
Hypoxylaceae
S
USA
Hanlin (1963)
Hypoxylon sp.*
Hypoxylaceae
E
China
Dissanayake et al. (2018)
Hysterium pulicare
(Lightf.) Pers.
Hysteriaceae
S
Italy
Greuter et al. (1991)
H. viticola Cooke & Peck
Hysteriaceae
S
USA
Saccardo (1878)
Hysterobrevium mori
(Schwein.) E. Boehm &
C.L. Schoch
Hysteriaceae
S
USA
Anonymous (1960), Barr
(1990), Tibpromma et al.
(2017)
Hysterographium
flexuosum Maire
Pleosporomycetidae
genera incertae
sedis
P, S
Stem lesions
USA
Hanlin (1963)
H. viticola (Cooke &
Peck) Rehm
Pleosporomycetidae
genera incertae
sedis
P, S
Stem lesions
USA
Wolf et al. (1938),
Anonymous (1960)
H. vulvatum (Schwein.)
Rehm
Pleosporomycetidae
genera incertae
sedis
P, S
Stem lesions
USA
Parris (1959), Anonymous
(1960)
Ilyonectria crassa
(Wollenw.) A. Cabral
& Crous*
Nectriaceae
P
Black foot
Uruguay
Abreo et al. (2010)
I. destructans
(Zinssmeister)
Rossman, L. Lombard
& Crous
Nectriaceae
P
Black foot
Argentina, Canada, France,
Iran, South Africa, Spain,
USA
Gerlach and Ershad (1970),
Seifert and Axelrood (1998),
Gatica et al. (2001), Petit
and Gubler (2005),
Gonzalez and Tello (2011),
Petit et al. (2011)
I. europaea A. Cabral,
Rego & Crous*
Nectriaceae
P
Black foot
Portugal
Úrbez-Torres et al. (2014),
Agusti-Brisach et al. (2016),
Carlucci et al. (2017)
I. liriodendri (Halleen,
Rego & Crous)
Chaverri & C. Salgado*
Nectriaceae
P
Black foot
Australia, Canada, France,
Portugal, South Africa,
Turkey, USA
Halleen et al. (2003), Petit
et al. (2011), WhitelawWeckert et al. (2013),
Úrbez-Torres et al. (2014),
Savas et al. (2015), AgustiBrisach et al. (2016)
I. lusitanica A. Cabral,
Rego & Crous*
Nectriaceae
P
Black foot
Portugal
Úrbez-Torres et al. (2014),
Agusti-Brisach et al. (2016),
Carlucci et al. (2017)
I. pseudodestructans A.
Cabral, Rego & Crous*
Nectriaceae
P
Black foot
Portugal
Úrbez-Torres et al. (2014),
Agusti-Brisach et al. (2016),
Carlucci et al. (2017)
123
Fungal Diversity (2018) 90:1–84
39
Table 6 (continued)
Species
Family
Life
mode
Disease caused
Locality
References
I. robusta (A.A. Hildebr.)
A. Cabral & Crous*
Nectriaceae
P
Black foot
Brazil, Canada, Portugal
Santos et al. (2014), ÚrbezTorres et al. (2014)
Ilyonectria sp.*
Nectriaceae
P, S
Black foot
Australia, China, Portugal
Úrbez-Torres et al. (2014),
Parkinson et al. (2017), This
study
Inocutis jamaicensis
(Murrill) A.M. Gottlieb,
J.E. Wright &
Moncalvo*
Hymenochaetaceae
P
Hoja de malvón
and chlorotic
leaf roll
Argentina, Uruguay
Abreo et al. (2012),
Rajchenberg and Robledo
(2013), Cloete et al. (2015)
Irpex lacteus (Fr.) Fr.
Phanerochaetaceae
E
USA
Brenckle (1918)
I. viticola
Phanerochaetaceae
S
USA
Saccardo (1878)
Kalmusia variispora
(Verkley, Göker &
Stielow) Ariyawansa &
K.D. Hyde
Didymosphaeriaceae
P
Syria
Verkley et al. (2014)
Karstenula yaline (Ellis
& Everh.) M.E. Barr
Didymosphaeriaceae
S
USA
Cash (1954)
Kazachstania viticola
Zubcova
Saccharomycetaceae
Kazakhstan
Zubkova (1971)
Kernia sp.*
Microascaceae
E, S
China
Dissanayake et al. (2018),
This study
Kluyveromyces
marxianus (E.C.
Hansen) Van der Walt
Saccharomycetaceae
P
Sour rot
Poland
Mulenko et al. (2008)
Kuehneola vitis (E.J.
Butler) Syd. & P. Syd.
Phragmidiaceae
P
Rust
India
Watson (1971), Ragunathan
and Ramakrishnan (1973)
Lachnella macrochaeta
Speg.
Niaceae
S
Italy
Farr (1973)
L. myceliosa W.B. Cooke
Niaceae
S
France, Germany
Batista and Ciferri (1962)
L. uvicola (Speg.) W.B.
Cooke
Niaceae
S
Argentina
Batista and Ciferri (1962)
Trunk disease
Fermented
juice
L.viticola Gonz. Frag.
Niaceae
S
Portugal
Unamuno (1941)
Lachnum virgineum
(Batsch) P. Karst.
Lachnaceae
S
Japan
Kobayashi (2007)
Lasiodiplodia brasiliense
M.S.B. Netto, M.W.
Marques & A.J.L.
Phillips*
Botryosphaeriaceae
P
Canker and die
back
Brazil
Correia et al. (2016b)
L. citricola
Abdollahzadeh, Javadi
& A.J.L. Phillips*
Botryosphaeriaceae
P
Canker and die
back
Italy
Carlucci et al. (2015)
L. crassispora T. Burgess
& Barber*
Botryosphaeriaceae
P
Canker and die
back
Brazil, South Africa, USA
Úrbez-Torres et al. (2010b),
van Niekerk et al. (2010),
Correia et al. (2013, 2016b)
L. egyptiaca A.M. Ismail,
L. Lombard & Crous*
Botryosphaeriaceae
P
Canker and die
back
Brazil
Correia et al. (2016b)
L. euphorbicola A.R.
Machado & O.L.
Pereira*
Botryosphaeriaceae
P
Canker and die
back
Brazil
Correia et al. (2016b)
L. hormozganensis
Abdollahzadeh, Zare &
A.J.L. Phillips*
Botryosphaeriaceae
P
Canker and die
back
Brazil
Correia et al. (2016b)
L. jatrophicola A.R.
Machado & O.L.
Pereira*
Botryosphaeriaceae
P
Canker and die
back
Brazil
Correia et al. (2016b)
123
40
Fungal Diversity (2018) 90:1–84
Table 6 (continued)
Species
Family
Life
mode
Disease caused
Locality
References
L. iraniensis
Abdollahzadeh, Zare &
A.J.L. Phillips*
Botryosphaeriaceae
P
Canker and die
back
Italy
Correia et al. (2016b), Netto
et al. (2017)
L. laeliocattleyae
(Sibilia) A. Alves*
Botryosphaeriaceae
P
Canker and die
back
Brazil
Correia et al. (2016b)
L. margaritacea Pavlic,
T.I. Burgess & M.J.
Wingf.*
Botryosphaeriaceae
S
China
This study
L. mediterranea
Linaldeddu, Deidda &
Berraf-Tebbal*
Botryosphaeriaceae
P
Canker and die
back
USA
Linaldeddu et al. (2015),
Cruywagen et al.(2017),
Netto et al. (2017)
L. missouriana ÚrbezTorres, Peduto &
Gubler*
Botryosphaeriaceae
P
Canker and die
back
Brazil, USA
Úrbez-Torres et al. (2012),
Netto et al. (2014, 2017),
Linaldeddu et al. (2015),
Trakunyingcharoen et al.
(2015), Correia et al.
(2016b), Cruywagen et al.
(2017), Coutinho et al.
(2017)
L. parva A.J.L. Phillips,
A. Alves & Crous*
Botryosphaeriaceae
P
Canker and die
back
Brazil
Correia et al. (2013)
L. plurivora Damm &
Crous*
Botryosphaeriaceae
P
Canker and die
back
Africa, South Africa
Damm et al. (2007), Begoude
et al. (2010), Doilom et al.
(2015), Coutinho et al.
(2017)
L. pseudotheobromae
A.J.L. Phillips, A.
Alves & Crous*
Botryosphaeriaceae
P
Canker and die
back
Brazil, China
Correia et al. (2013, 2016b),
Dissanayake et al. (2015)
L. theobromae (Pat.)
Griffon & Maubl.*
Botryosphaeriaceae
P, E
Canker and die
back
Argentina, Australia, Bolivia,
Brazil, China, Egypt, Florida,
Iran, Italy, Iraq, Portugal,
South Africa, Spain, Turkey,
Uganda, USA
Alfieri Jr. et al. (1984), ÚrbezTorres et al. (2006), van
Niekerk et al. (2006), Pitt
et al. (2010), Qiu et al.
(2011), Yan et al. (2011b),
Mondello et al. (2013),
Dissanayake et al. (2018)
L. viticola Úrbez-Torres,
Peduto & Gubler*
Botryosphaeriaceae
P
Canker and die
back
USA
Úrbez-Torres et al. (2012),
Linaldeddu et al. (2015),
Comont et al. (2016),
Coutinho et al. (2017), Netto
et al. (2017)
L. vitis Tao Yang &
Crous*
Botryosphaeriaceae
P
Canker and die
back
Italy
Yang et al. (2017)
Lasiodiplodia sp.*
Botryosphaeriaceae
P, S,
E
Canker and die
back
China, Italy
Mondello et al. (2013),
Dissanayake et al. (2018),
This study
Lecanicillium lecanii
(Zimm.) Zare & W.
Gams
Cordycipitaceae
E
Spain
Gonzalez and Tello (2011)
Lecanicillium sp.*
Cordycipitaceae
S
China
This study
Lecanidion atratum
(Hedw.) Endl.
Patellariaceae
S
Italy
Greuter et al. (1991)
Lecythophora hoffmannii
(J.F.H. Beyma) W.
Gams & McGinnis*
Coniochaetaceae
E
Switzerland
Casieri et al. (2009)
Lentinus sp.*
Polyporaceae
S
China
This study
Lenzites betulina (L.) Fr.
Polyporaceae
S
Pakistan
Ahmad et al. (1997)
123
Fungal Diversity (2018) 90:1–84
41
Table 6 (continued)
Species
Family
Life
mode
Disease caused
Locality
References
Black rot
Leptodothiorella sp.
Botryosphaeriaceae
P
Russia
Melnik and Popushoi (1992)
Leptosphaeria ampelina
Curzi & Barbaini
Leptosphaeriaceae
E
Italy
Crane and Shearer (1991)
L. cerlettii Speg.
Leptosphaeriaceae
S
Italy
Farr (1973), Crane and
Shearer (1991)
L. chaetostoma Sacc.
Leptosphaeriaceae
S
Italy
Crane and Shearer (1991)
L. cirricola Pass.
Leptosphaeriaceae
S
Italy
Crane and Shearer (1991)
L. gibelliana Pirotta
Leptosphaeriaceae
S
Italy
Crane and Shearer (1991)
L. ogilviensis (Berk. &
Broome) Ces. & De
Not.
Leptosphaeriaceae
S
Pakistan
Ahmad (1978)
L. pampini (Thüm.) Sacc.
Leptosphaeriaceae
S
France, Italy, Portugal
Unamuno (1941), Crane and
Shearer (1991)
L. yalin Sacc.
Leptosphaeriaceae
S
Italy, UK
Cannon et al. (1985), Crane
and Shearer (1991)
L. vagabunda Sacc.
L. vinealis Pass.
Leptosphaeriaceae
Leptosphaeriaceae
S
S
USA
Italy
Hanlin (1963)
Crane and Shearer (1991)
L. viticola Fautrey &
Roum.
Leptosphaeriaceae
S
France
Crane and Shearer (1991)
L. vitigena Sacc.
Leptosphaeriaceae
S
Austria
Crane and Shearer (1991)
L. vitis (Castagne) Pirotta
Leptosphaeriaceae
S
Austria, France
Crane and Shearer (1991)
Leptosphaeria sp.*
Leptosphaeriaceae
E, S
China, Spain, Switzerland,
Venezuela
Urtiaga (1986), Casieri et al.
(2009), Gonzalez and Tello
(2011), This study
Leptothyrium passerinii
Thüm.
Ascomycota genera
incertae sedis
E
China
Tai (1979)
Leucostoma persoonii
(Nitschke) Höhn.*
Valsaceae
P
Canker
Germany, Italy, Spain
Greuter et al. (1991), Fischer
et al. (2016)
Libertella blepharis A.L.
Sm.
Diatrypaceae
P, E
Trunk disease
Bulgaria
Bobev (2009)
L. viticola Fautrey
Diatrypaceae
E
France
Fautrey and Lambotte (1896)
Libertella sp.
Diatrypaceae
P, E
Australia, Spain
Sosnowski et al. (2007),
Gonzalez and Tello (2011)
Lophidium nitidum Ellis
& Everh.
Lophiostomataceae
S
USA
Cash (1953)
Lophiostoma caulium
(Fr.) Ces. & De Not.
Lophiostomataceae
E
Poland
Mulenko et al. (2008)
Trunk disease
L. elegans (Fabre) Sacc.
Lophiostomataceae
E
Pakistan
Ahmad (1969)
L. macrostomum (Tode)
Ces. & De Not.*
Lophiostomataceae
E, S
Pakistan, Italy
Ahmad (1978), Ahmad et al.
(1997), This study,
Jayawardena et al. (2018)
L. pustulatum Ellis &
Everh.
Lophiostomataceae
E
USA
Cash (1953)
L. rhopalosporum Ellis &
Everh.
Lophiostomataceae
E
USA
Cash (1953)
L. scrophulariae Peck
Lophiostomataceae
E
Canada, USA
Barr (1992)
L. stenostomum Ellis &
Everh.
L. subcorticale Fuckel
Lophiostomataceae
E
USA
Cash (1953)
Lophiostomataceae
E
Italy
Saccardo (1878)
L. thuemenianum Speg.
Lophiostomataceae
E
Italy
Farr (1973)
123
42
Fungal Diversity (2018) 90:1–84
Table 6 (continued)
Species
Family
Life
mode
L. vitigenum (Kaz.
Tanaka & Y. Harada)
K. Hirayama & Kaz.
Tanaka
Lophiostomataceae
Lophiostoma sp.*
Locality
References
E
Japan
Hirayama and Tanaka (2011)
Lophiostomataceae
E, S
China
Dissanayake et al. (2018),
This study
Lophiotrema eburnoides
Kaz. Tanaka, A.
Hashim. & K. Hiray.*
Lophiotremataceae
S
Japan
Liu et al. (2015)
L. vitigenum Kaz. Tanaka
& Y. Harada
Lophiotremataceae
S
Japan
Tanaka and Harada (2003),
Kobayashi (2007)
Loranitschkia viticola
Lar.N. Vassiljeva
Nitschkiaceae
S
China, Kunashir Island, Russia
Vasilyeva (1990), Vasilyeva
et al. (2009, 2010)
Macrophoma farlowiana
(Viala & Sauv.) Tassi
Botryosphaeriaceae
P
Macrophoma
rot
USA
Anonymous (1960), Greene
(1966)
M. flaccida (Viala &
Ravaz) Cavara
Botryosphaeriaceae
P
Macrophoma
rot
Bulgaria, France, Greece, India,
Italy, Portugal
Mathur (1979), Phillips and
Lucas (1997), Phillips
(2000), Bobev (2009)
M. longispora (I.
Miyake) Hara
Botryosphaeriaceae
P
Macrophoma
rot
USA
Anonymous (1960)
M. peckiana Dearn. &
House
Botryosphaeriaceae
P
Macrophoma
rot
USA
Anonymous (1960)
M. reniformis (Viala &
Ravaz) Cavara
Botryosphaeriaceae
P
Macrophoma
rot
Italy, USA
Anonymous (1960), Phillips
and Lucas (1997)
M. rimiseda (Sacc.) Berl.
& Voglino
Botryosphaeriaceae
P
Macrophoma
rot
Greece, Morocco, Turkey
Watson (1971), Pantidou
(1973)
M. sicula Scalia
Botryosphaeriaceae
P
Macrophoma
rot
Central Asia, Italy
Koshkelova and Frolov
(1973), Greuter et al. (1991)
Macrophoma sp.
Botryosphaeriaceae
P
Macrophoma
rot
India, USA
Mathur (1979), Alfieri Jr.
et al. (1984)
Macrophomina
phaseolina (Tassi)
Goid.
Botryosphaeriaceae
P, E
Charcoal rot
Australia, Hawaii, India,
Malawi, South Africa, Spain,
Peregrine and Siddiqi (1972),
Marais (1979), Raabe et al.
(1981), Gonzalez and Tello
(2011)
Macrosporium vitis
(Cavara) Cavara
Pleosporaceae
E
Chile
Mujica and Vergara (1945)
Macrosporium sp.
Pleosporaceae
E
Bulgaria, Greece, South Africa
Alexopoulos (1940), Doidge
(1950), Bobev (2009)
Marssonina viticola (I.
Miyake) F.L. Tai
Drepanopezizaceae
E
China, Japan, Taiwan
Sawada (1959), Watson
(1971), Tai (1979),
Kobayashi (2007)
Marasmius sp.*
Marasmiaceae
S
China
This study
Massariella viticola
Frolov
Amphisphaeriaceae
S
Central Asia
Koshkelova and Frolov (1973)
Massarina corticola
(Fuckel) L. Holm*
Massarinaceae
S
Switzerland
Casieri et al. (2009)
Merismodes bresadolae
(Grélet) Singer
Niaceae
E
Italy
Farr (1973)
Meliola vitis Hansf.
Meliolaceae
E
India, Uganda
Hansford (1947), Patil and
Mahamulkar (1999)
Metarhizium sp.*
Clavicipitaceae
S
China
This study
Metasphaeria social
(Sacc.) Sacc.
Dothioraceae
S
Italy
Greuter et al. (1991)
123
Disease caused
Fungal Diversity (2018) 90:1–84
43
Table 6 (continued)
Species
Family
Life
mode
Metschnikowia
pulcherrima Pitt &
M.W. Mill.
Metschnikowiaceae
M. viticola G. Péter,
Tornai-Leh., M. Suzuki
& Dlauch*
Disease caused
Locality
References
E
USA
Batra (1973)
Metschnikowiaceae
E
Hungary
Peter et al. (2005)
Microascus brevicaulis
S.P. Abbott*
Helotiales genera
incertae sedis
E
China
Dissanayake et al. (2018)
Microascus sp.
Helotiales genera
incertae sedis
S
China
This study
Microdochium bolleyi (R.
Sprague) de Hoog &
Herm. Nijh.*
Microdochiaceae
E
Switzerland
Casieri et al. (2009)
Microdochium sp.*
Microdochiaceae
S
China
This study
Microdiplodia
microsporella (Sacc.)
Allesch.
Ascomycota genera
incertae sedis
P
Poland
Mulenko et al. (2008)
M. vineae (Pass. &
Beltrani) Tassi
Ascomycota genera
incertae sedis
S
Italy
Tassi (1902), Greuter et al.
(1991)
Micropera ampelina
Sacc. & Fairm.
Ascomycota genera
incertae sedis
S
USA
Anonymous (1960)
Microthyrium
microscopicum Desm.
Microthyriaceae
S
Portugal
Unamuno (1941)
Minimedusa sp.*
Cantharellales
incertae sedis
S
China
This study, Jayawardena et al.
(2018)
Moeszia cylindroides
Bubák
Nectriaceae
S
Japan
Tubaki (1958)
Mollisia cinerea (Batsch)
P. Karst.
Mollisiaceae
S
USA
Hanlin (1963)
M. melaleuca (Fr.) Sacc.
M. pullata (W.R. Gerard)
Dennis
Mollisiaceae
Mollisiaceae
S
S
USA
USA
Hanlin (1963)
Dennis (1964)
Monilinia fructicola (G.
Winter) Honey*
Sclerotiniaceae
P
Canada, Japan, New Zealand,
USA
Preston (1945), Pennycook
(1989), Kobayashi (2007),
Hrustic et al. (2015)
M. fructigena (Pers.)
Pers.
Sclerotiniaceae
S
China
Tai (1979)
M. laxa (Aderh. &
Ruhland) Honey
Sclerotiniaceae
S
New Zealand
Pennycook (1989)
Monochaetia
ampelophila Speg.
Xylariomycitidae
genera insertae
sedis
E
Argentina
Guba (1961), Nag Raj (1993)
M. uniseta (Tracy &
Earle) Sacc. & D. Sacc.
Xylariomycitidae
genera insertae
sedis
E
USA
Nag Raj (1993)
Monochaetinula
ampelophila (Speg.)
Nag Raj
Ascomycota genera
incertae sedis
E
Argentina
Nag Raj (1993)
M. terminaliae (Bat. &
J.L. Bezerra)
Muthumary, Abbas &
B. Sutton
Ascomycota genera
incertae sedis
E
India
Muthumary et al. (1986)
Monodictys antiqua
(Corda) S. Hughes
Dothideomycetes
genera incertae
sedis
S
Portugal
de Sousa Dias and Lucas
(1972)
Trunk disease
Brown rot
123
44
Fungal Diversity (2018) 90:1–84
Table 6 (continued)
Species
Family
Life
mode
Mortierella hyalina
(Harz) W. Gams*
Mortierellaceae
Mortierella sp.*
Locality
References
S
Switzerland
Casieri et al. (2009)
Mortierellaceae
E, S
China
Dissanayake et al. (2018),
This study
Mucor circinelloides
Tiegh.*
Mucoraceae
S
China, Switzerland
M. hiemalis Wehmer*
Mucoraceae
E, S
Spain, Switzerland
Casieri et al. (2009), This
study, Jayawardena et al.
(2018)
Casieri et al. (2009), Gonzalez
and Tello (2011)
M. moelleri (Vuill.)
Lendn.*
Mucoraceae
S
Switzerland
Casieri et al. (2009)
M. plumbeus Bonord.*
Mucoraceae
S
Switzerland
Casieri et al. (2009)
M. racemosus Fresen.*
Mucoraceae
E, S
China, Spain, Switzerland
Casieri et al. (2009), Gonzalez
and Tello (2011), This
study, Jayawardena et al.
(2018)
Mucor sp.
Mucoraceae
E
Greece, Spain, USA
Pantidou (1973), Shaw
(1973), Gonzalez and Tello
(2011)
Mycosphaerella
cuboniana (D. Sacc.)
Tomilin
Mycosphaerellaceae
P
Greece
Pantidou (1973)
M. graminicola (Fuckel)
J. Schröt*
Mycosphaerellaceae
E
China
Dissanayake et al. (2018)
M. manganottiana (C.
Massal.) Tomilin
Mycosphaerellaceae
P
Leaf spot
Greece
Pantidou (1973)
M. vitis (Fuckel) J.
Schröt.
Mycosphaerellaceae
P
Leaf spot
Japan, Poland, Russia
Watson (1971), Kobayashi
(2007), Mulenko et al.
(2008)
Mycosphaerella sp.*
Mycosphaerellaceae
E
China, USA, Venezuela
Stevenson and Wellman
(1944), Dissanayake et al.
(2018)
Myrothecium sp.*
Stachybotryaceae
P, S
China, USA
Alfieri Jr. et al. (1984), This
study
Myxosporium viticola
Dearn. & House
Ascomycota genera
incertae sedis
S
USA
Anonymous (1960)
Nectria cinnabarina
(Tode) Fr.
Nectriaceae
S
USA
Seifert (1985), Anonymous
(1960), Shaw (1973)
N. ramulariae
(Wollenw.) E. Müll.*
Nectriaceae
P, E
Spain, Switzerland
Casieri et al. (2009), Gonzalez
and Tello (2011)
Nectria sp.
Nectriaceae
S
Korea, Mexico
Alvarez (1976), Cho and Shin
(2004)
Nemania serpens (Pers.)
Gray
Xylariaceae
E
Spain
Gonzalez and Tello (2011)
Neoanthostomella
viticola Daranagama,
Camporesi & K.
D. Hyde*
Xylariaceae
S
Italy
Daranagama et al. (2016),
This study, Jayawardena
et al. (2018)
Neofusicoccum
algeriense BerrafTebbal & A.J.L.
Phillips*
Botryosphaeriaceae
P
Algeria
Berraf-Tebbal et al. (2014),
Nogueira et al. (2016)
123
Disease caused
Leaf spot
Leaf spot
Canker, die
back
Fungal Diversity (2018) 90:1–84
45
Table 6 (continued)
Species
Family
Life
mode
Disease caused
Locality
References
N. australe (Slippers,
Crous & M.J. Wingf.)
Crous, Slippers &
A.J.L. Phillips*
Botryosphaeriaceae
P
Canker, die
back
Algeria, Australia, Chile, Italy,
Mexico, New Zealand, South
Africa, Spain, Uruguay, USA
van Niekerk et al.
(2004a, b, 2006), Luque
et al. (2005), Phillips et al.
(2005), Taylor et al. (2005),
Úrbez-Torres et al. (2006),
Cunnington et al. (2007),
Baskarathevan et al. (2008),
Úrbez-Torres (2011), Martin
et al. (2011b), Sessa et al.
(2016)
N. cordaticola Pavlic,
Slippers & M.J.
Wingf.*
Botryosphaeriaceae
P
Canker, die
back
Italy
Sakalidis et al. (2013)
N.italicum Dissan. &
K.D. Hyde*
Botryosphaeriaceae
S
Italy
Marin-Felix et al. (2017)
N. kwambonambiense
Pavlic, Slippers & M.J.
Wingf.*
Botryosphaeriaceae
P
Canker, die
back
Uruguay
Sessa et al. (2016)
N. luteum (Pennycook &
Samuels) Crous,
Slippers & A.J.L.
Phillips*
Botryosphaeriaceae
P
Botryosphaeria
die back
Australia, Germany, Italy, New
Zealand, Portugal, South
Africa, Spain, Tunisia,
Uruguay, USA
Pennycook (1989), van
Niekerk et al. (2004a, b),
Luque et al. (2005, 2009),
Úrbez-Torres et al. (2007),
Baskarathevan et al. (2008),
Abreo et al. (2012), Fischer
et al. (2016)
N. macroclavatum (T.I.
Burgess, Barber & G.E.
Hardy) T.I. Burgess,
Barber & G.E. Hardy
Botryosphaeriaceae
P
Canker, die
back
New Zealand
Billones et al. (2010), ÚrbezTorres (2011)
N. mangiferae (Syd. & P.
Syd.) Crous, Slippers &
A.J.L. Phillips*
Botryosphaeriaceae
P
Canker, die
back
China
Dissanayake et al. (2015)
N. mediterraneum Crous,
M.J. Wingf. & A.J.L.
Phillips*
Botryosphaeriaceae
P
Canker, die
back
Algeria, Spain, USA
Úrbez-Torres et al.
(2010a, b, c), Berraf-Tebbal
et al. (2014)
N. occulatum Sakalidis &
T.I. Burgess*
Botryosphaeriaceae
P
Canker, die
back
Australia
Sakalidis et al. (2013)
N. parvum (Pennycook &
Samuels) Crous,
Slippers & A.J.L.
Phillips*
Botryosphaeriaceae
P, E,
S
Botryosphaeria
die back
Australia, Italy, Brazil, Canada,
Chile, China, France, New
Zealand, Portugal, South
Africa, Spain, Switzerland,
Uruguay, USA
Phillips et al. (2002, 2005),
van Niekerk et al.
(2004a, b, 2006), Luque
et al. (2005, 2009), ÚrbezTorres et al. (2006),
Cunnington et al. (2007),
Baskarathevan et al. (2008),
Casieri et al. (2009),
Gonzalez and Tello (2011),
Abreo et al. (2012), Correia
et al. (2013), Mondello et al.
(2013), Sakalidis et al.
(2013), Wu et al. (2015),
This study, Jayawardena
et al. (2018)
123
46
Fungal Diversity (2018) 90:1–84
Table 6 (continued)
Species
Family
Life
mode
Disease caused
Locality
References
N. ribis (Slippers, Crous
& M.J. Wingf.) Crous,
Slippers & A.J.L.
Phillips
Botryosphaeriaceae
P
Botryosphaeria
die back,
Macrophoma
rot
Australia, Italy, South Africa,
Tanzania, Pakistan, Portugal,
USA
Anonymous (1960), Ebbels
and Allen (1979),
Milholland (1994), Ahmad
et al. (1997), Phillips (2000),
Halleen et al. (2003), van
Niekerk et al. (2006)
N. stellenboschiana Tao
Yang & Crous*
Botryosphaeriaceae
P
Canker, die
back
South Africa
Yang et al. (2017)
N. viticlavatum (Van
Niekerk & Crous)
Crous, Slippers &
A.J.L. Phillips
Botryosphaeriaceae
P
Canker, die
back
South Africa
Burgess et al. (2005), Farr
et al. (2005), Luque et al.
(2005), Phillips et al. (2005),
van Niekerk et al. (2006)
N. vitifusiforme (Van
Niekerk & Crous)
Crous, Slippers &
A.J.L. Phillips
Botryosphaeriaceae
P
Botryosphaeria
die back
Italy, Mexico, South Africa,
Spain, USA
van Niekerk et al. (2004a, b),
Burgess et al. (2005), Luque
et al. (2009), CandolfiArballo et al. (2010), ÚrbezTorres (2011), Mondello
et al. (2013)
Neomassaria fabacearum
Mapook, Camporesi &
K.D. Hyde*
Massariaceae
S
Italy
This study, Jayawardena et al.
(2018)
Neonectria candida
(Ehrenb.) Rossman, L.
Lombard & Crous*
N. coccinea (Pers.)
Rossman & Samuels
Nectriaceae
S
Spain, Switzerland
Casieri et al. (2009), Gonzalez
and Tello (2011)
Nectriaceae
S
USA
Anonymous (1960)
N. fuckeliana (C. Booth)
Castl. & Rossman*
Nectriaceae
P, E
Canada, Spain, Switzerland
Casieri et al. (2009), Gonzalez
and Tello (2011), Petit et al.
(2011)
N. macrodidyma Halleen,
Schroers & Crous*
Nectriaceae
S
Switzerland
Casieri et al. (2009)
N. microconidia J. Luo,
P. Zhao & W.Y.
Zhuang*
Nectriaceae
S
Japan
Hirooka et al. (2013)
N. obtusispora (Cooke &
Harkn.) Rossman, L.
Lombard & Crous
Nectriaceae
P
Black-foot
disease
Italy, USA
Scheck et al. (1998a, b),
Greuter et al. (1991)
Neopestalotiopsis
asiatica (Maharachch.
& K.D. Hyde)
Maharachch., K.D.
Hyde & Crous*
Sporocadaceae
P
Leaf stripe
France
Maharachchikumbura et al.
(2016)
N. clavispora (G.F. Atk.)
Maharachch., K.D.
Hyde & Crous*
Sporocadaceae
S
China
This study, Jayawardena et al.
(2018)
N. javaensis
Maharachch., K.D.
Hyde & Crous*
Sporocadaceae
E
France
Maharachchikumbura et al.
(2016)
N. vitis Jayawardena,
Maharachch., Yan, Li
& Hyde*
Sporocadaceae
P, S
Fruit rot, trunck
disease, leaf
spot
China
Jayawardena et al. (2016a, b)
Neopestalotiopsis sp.*
Sporocadaceae
P
Leaf spot
China, France, India
Jayawardena et al. (2015),
Maharachchikumbura et al.
(2014, 2016)
Neoplaconema sp.*
Ascomycota genera
incertae sedis
P
Switzerland
Casieri et al. (2009)
123
Fungal Diversity (2018) 90:1–84
47
Table 6 (continued)
Species
Family
Life
mode
Disease caused
Locality
References
Neoscytalidium
dimidiatum (Penz.)
Crous & Slippers*
Botryosphaeriaceae
P
Wood canker,
die back
Brazil, India, Iraq, USA,
Wangikar et al. (1969),
Sarbhoy et al. (1971),
Mathur (1979), Al-Saadoon
et al. (2012), Rolshausen
et al. (2013), Correia et al.
(2016a)
Neurospora sp.*
Sordariaceae
S
China
This study
Nigrospora oryzae (Berk.
& Broome) Petch*
Sordariomycetes
genera incertae
sedis
E
China, Spain
Gonzalez and Tello (2011),
Dissanayake et al. (2018)
N. sphaerica (Sacc.)
E.W. Mason*
Sordariomycetes
genera incertae
sedis
E
China
Dissanayake et al. (2018)
Nodulisporium sp.
Xylariaceae
E
Spain
Gonzalez and Tello (2011)
Oidiodendron sp.*
Myxotrichaceae
E
China
Dissanayake et al. (2018)
Ophiocordyceps sp.*
Ophiocordycipitaceae
S
China
This study
Ophiostoma piceae
(Münch) Syd. & P.
Syd.*
Ophiostomataceae
E
Spain, Switzerland
Casieri et al. (2009), Gonzalez
and Tello (2011)
O. quercus (Georgev.)
Nannf.*
Ophiostomataceae
E
Switzerland
Casieri et al. (2009)
O. subalpinum Ohtaka &
Masuya*
Ophiostomataceae
E
Switzerland
Casieri et al. (2009)
Ophiostoma sp.*
Ostreichnion curtisii
(Duby) M.L. Lohman
Ophiostomataceae
Hysteriaceae
E
S
Switzerland
USA
Casieri et al. (2009)
Hanlin (1963)
Ostreola viticola R. Rao
& Modak
Mytilinidiaceae
S
India
Pande (2008)
Paecilomyces sp.
Thermoascaceae
P
Root stock
South Africa
Halleen et al. (2003)
Papiliotrema laurentii
(Kuff.) X.Z. Liu, F.Y.
Bai, M. Groenew. &
Boekhout
Tremellaceae
P
Melting decay
USA
Morgan and Michailides
(2004)
Papulospora sp.*
Sordariomycetes
genera incertae
sedis
S
China
This study
Pareutypella sulcata
Y.M. Ju & J.D. Rogers
Sordariomycetes
genera incertae
sedis
S
Taiwan
Ju and Rogers (1995)
Passalora dissiliens
(Duby) U. Braun &
Crous
Mycosphaerellaceae
P
Leaf spot
Australia, Bulgaria, China,
Egypt, France, Iran, India.
Israel, Japan, South Africa,
Pakistan, Palestine, Poland,
Portugal, Yemen
Crous and Braun (2003), Guo
and Liu (2003), Zhuang
(2005), Kobayashi (2007),
Bobev (2009), Mouchacca
(2009)
P. fulva (Cooke) U.
Braun & Crous*
Mycosphaerellaceae
P
Leaf spot
Switzerland
Casieri et al. (2009)
P. heterosporella U.
Braun & Crous
Mycosphaerellaceae
P
Leaf spot
Israel, USA
Crous and Braun (2003)
P. vitis (M.S. Patil &
Sawant) Poonam
Srivast.
Mycosphaerellaceae
P
Leaf spot
India
Crous and Braun (2003),
Kamal (2010)
P. vitis-piadezkii U.
Braun & Crous
Mycosphaerellaceae
P
Leaf spot
China
Crous and Braun (2003), Guo
and Liu (2003)
123
48
Fungal Diversity (2018) 90:1–84
Table 6 (continued)
Species
Family
Life
mode
Disease caused
Locality
References
P. vitis-ripariae (U.
Braun) U. Braun &
Crous
Mycosphaerellaceae
P
Leaf spot
USA
Crous and Braun (2003)
Patellaria atrata (Hedw.)
Fr.
Patellariaceae
S
Central Asia
Koshkelova and Frolov (1973)
P. lantanae R. Rao
Patellariaceae
S
India
Pande (2008)
P. viticola Pers.
Patellariaceae
S
Spain
Unamuno (1941)
Paraphoma
chrysanthemicola
(Hollós) Gruyter,
Aveskamp & Verkley*
Phaeosphaeriaceae
S
China
This study, Jayawardena et al.
(2018)
Penicillium
adametzioides S. Abe
Aspergillaceae
E, S
Japan
Kobayashi (2007)
P. astrolabium R. Serra
& S.W. Peterson*
Aspergillaceae
S
Portugal
Serra and Peterson (2007)
P. aurantiogriseum
Dierckx
Aspergillaceae
P
South Africa
Gorter (1977)
P. brevicompactum
Dierckx*
Aspergillaceae
S
China
This study, Jayawardena et al.
(2018)
P. chrysogenum Thom*
Aspergillaceae
S
China
This study
P. citrinum Thom*
Aspergillaceae
S
China
This study, Jayawardena et al.
(2018)
P. digitatum (Pers.)
Sacc.*
Aspergillaceae
E
China
Dissanayake et al. (2018)
Fruit rot
P. elongatum Dierckx
Aspergillaceae
P
Fruit rot
South Africa
Gorter (1977)
P. expansum Link
Aspergillaceae
P
Fruit rot
Bulgaria, South Africa, USA
Gorter (1977), Bobev (2009)
P. funiculosum Thom
Aspergillaceae
S
Cyprus
Georghiou and Papadopoulos
(1957)
P. italicum Wehmer
Aspergillaceae
P
Greece
Pantidou (1973)
P. neocrassum R. Serra &
S.W. Peterson*
Aspergillaceae
S
Portugal
Serra and Peterson (2007)
P. olsonii Bainier &
Sartory*
P. rolfsii Thom
Aspergillaceae
E
Portugal
Serra and Peterson (2007)
Aspergillaceae
E
USA
Shaw (1973)
Aspergillaceae
S
Japan
Kobayashi (2007)
P. sclerotigenum W.
Yamam.
Fruit rot
P. sumatraense Svilv.*
Aspergillaceae
P
Iran
Mahdian and Zafari (2017)
P. terrigenum
Houbraken, Frisvad &
Samson*
Aspergillaceae
S
China
This study, Jayawardena et al.
(2018)
P. toxicarium I. Miyake*
Aspergillaceae
P, E
Spain
Garcia-Benavides et al. (2013)
P. variabile Sopp
Aspergillaceae
S
Penicillium sp.*
Aspergillaceae
P, E,
S
123
Fruit rot
Fruit rot
USA
Shaw (1973)
Australia, Chile, China, Cuba,
France, Italy, Japan, Korea,
South Africa, Spain,
Switzerland, USA
French (1989), Castillo-Pando
et al. (2001), Fourie and
Halleen (2002), Casieri et al.
(2009), Gonzalez and Tello
(2011), Mondello et al.
(2013), Oh et al. (2014),
Dissanayake et al. (2018),
This study
Fungal Diversity (2018) 90:1–84
49
Table 6 (continued)
Species
Family
Life
mode
Peniophora
albomarginata
(Schwein.) Massee
Peniophoraceae
P. viticola (Schwein.)
Höhn. & Litsch.
Disease caused
Locality
References
S
USA
Hanlin (1966)
Peniophoraceae
S
USA
Hanlin (1966)
Peniophora sp.*
Peniophoraceae
S
China
Penzigomyces dissolvens
(Hol.-Jech., Mercado &
J. Mena) J. Mena*
Ascomycota genera
incertae sedis
S
Cuba
This study, Jayawardena et al.
(2018)
Mena-Portales et al. (2000)
Perenniporia tenuis
(Schwein.) Ryvarden
P. unita (Pers.) Murrill
Polyporaceae
S
Greece
Polyporaceae
S
USA
Periconia byssoides Pers.
Periconiaceae
E
Argentina, USA
Grand (1985), Carmaran and
Novas (2003)
P. igniaria E.W. Mason
& M.B. Ellis
Periconiaceae
E
Spain
Gonzalez and Tello (2011)
Pestalotiopsis biciliata
Maharachch., K.D.
Hyde & Crous*
Sporocadaceae
P
France
Maharachchikumbura et al.
(2016)
P. chamaeropis
Maharachch., K.D.
Hyde & Crous*
Sporocadaceae
S
Italy
This study, Jayawardena et al.
(2018)
P. funerea (Desm.)
Steyaert
Sporocadaceae
P
Leaf spot
Japan
Kobayashi (2007)
P. mangiferae (Henn.)
Steyaert
Sporocadaceae
P
Leaf spot
Myanmar
Thaung (2008c)
P. menezesiana (Bres. &
Torrend) Bissett*
Sporocadaceae
P
Fruit rot
Australia, China, Greece, India,
Japan, Madeira Islands, USA
Mundkur and Thirumalachar
(1946), Alfieri Jr. et al.
(1984, Nag Raj (1993),
Sergeeva et al. (2005)
P. quadriciliata (Bubák
& Dearn.) Bissett
Sporocadaceae
P
Leaf spot
Canada
Nag Raj (1993)
P. trachicarpicola Y.M.
Zhang & K.D. Hyde*
Sporocadaceae
P
Fruit rot, trunck
disease
China
Jayawardena et al. (2015)
P. uvicola (Speg.)
Bissett*
Sporocadaceae
P
Fruit rot
Australia, China, India, Italy,
Japan, Korea, USA
Simmonds (1966), Tai (1979),
Nag Raj (1988, 1993), Cho
and Shin (2004), Sergeeva
et al. (2005), Kobayashi
(2007), Ge et al. (2009),
Maharachchikumbura et al.
(2011), Úrbez-Torres et al.
(2012)
Pestalotiopsis sp.*
Sporocadaceae
P, E,
S
Fruit rot
Australia, Cuba, Italy, Japan,
Korea, South Africa, USA
Urtiaga (1986), Halleen et al.
(2003), Castillo-Pando et al.
(2001), Úrbez-Torres et al.
(2012), This study
Leaf stripe,
defoliated
shoots
Kotlaba (1997), Zervakis et al.
(1998)
Hanlin (1966)
123
50
Fungal Diversity (2018) 90:1–84
Table 6 (continued)
Species
Family
Life
mode
Disease caused
Locality
References
Phaeoacremonium
aleophilum W. Gams,
Crous, M.J. Wingf. &
Mugnai*
Togniniaceae
P, E
Esca
Algeria, Argentina, Austria,
Australia, France, Italy, Iran,
Serbia, South Africa, Spain,
Turkey, Uruguay, USA,
Yugoslavia
Larignon and Dubos (1997),
Pascoe and Cottral (2000),
Gatica et al. (2001), Lardner
et al. (2005), Whiting et al.
(2005), Mostert et al.
(2006), Sosnowski et al.
(2007), Luque et al. (2009),
Berraf-Tebbal et al. (2011),
Gonzalez and Tello (2011),
Abreo et al. (2012),
Mohammadi and
Banihashemi (2012),
Garcia-Benavides et al.
(2013), Mohammadi et al.
(2013a), Úrbez-Torres et al.
(2013a, b)
P. alvesii L. Mostert,
Summerb. & Crous*
Togniniaceae
P
Esca
South Africa, Turkey
Essakhi et al. (2008), White
et al. (2011)
P. amstelodamense L.
Mostert, Summerb. &
Crous
Togniniaceae
P
Esca
Netherland
Arzanlou et al. (2014)
P. angustius W. Gams,
Crous & M.J. Wingf.
Togniniaceae
P
Esca
France, Portugal, USA
Chicau et al. (2000), Whiting
et al. (2005)
P. argentinense L.
Mostert, W. Gams &
Crous*
Togniniaceae
P
Esca
Argentina
Arzanlou et al. (2014)
P. armeniacum A.B.
Graham, P.R. Johnst. &
B. Weir*
Togniniaceae
P
Esca
New Zealand
Graham et al. (2009),
Arzanlou et al. (2014),
Úrbez-Torres et al. (2014)
P. australiense L.
Mostert, Summerb. &
Crous*
Togniniaceae
P
Esca
Australia, Uruguay
Mostert et al. (2006), Graham
et al. (2009), Abreo et al.
(2012), Arzanlou et al.
(2014), Úrbez-Torres et al.
(2014)
P. austroafricanum L.
Mostert, W. Gams &
Crous*
Togniniaceae
P
Esca
South Africa
Berraf-Tebbal et al. (2011),
Úrbez-Torres et al. (2014)
P. canadense J.R. ÚrbezTorres, P. Haag & D.T.
O’Gorman*
Togniniaceae
P
Esca
Canada
Úrbez-Torres et al. (2014)
P. chlamydospora (W.
Gams, Crous, M.J.
Wingf. & Mugnai)
Crous & W. Gams*
Togniniaceae
P
Esca
Australia, Chile, France, Italy,
Portugal, South Africa, USA
Larignon and Dubos (1997),
Dupont et al. (1998), Scheck
et al. (1998b), Chicau et al.
(2000), Pascoe and Cottral
(2000), Auger et al. (2004b),
Lardner et al. (2005), Santos
et al. (2006)
P. cinereum Gramaje,
Mohammadi,
Banihashemi,
Armengol & L.
Mostert*
Togniniaceae
P
Esca
Iran
Gramaje et al. (2009),
Mohammadi and
Banihashemi (2012),
Mohammadi et al. (2013a),
Úrbez-Torres et al. (2014),
Sami et al. (2014)
P.
fraxinopennsylvanicum
(T.E. Hinds) D.
Gramaje, L. Mostert &
Crous*
Togniniaceae
P
Esca
Canada, Croatia, Germany,
Hungary, Iran, South Africa,
Spain, USA
Eskalen et al. (2005), Fischer
et al. (2016)
123
Fungal Diversity (2018) 90:1–84
51
Table 6 (continued)
Species
Family
Life
mode
Disease caused
Locality
References
P. globosum A.B.
Graham, P.R. Johnst. &
B. Weir*
Togniniaceae
P
Esca
New Zealand
Graham et al. (2009),
Arzanlou et al. (2014),
Úrbez-Torres et al. (2014)
P. griseorubrum L.
Mostert, Summerb. &
Crous*
Togniniaceae
P
Esca
Italy
Essakhi et al. (2008), Gramaje
et al. (2009), Berraf-Tebbal
et al. (2011)
P. hispanicum Gramaje,
Armengol & L.
Mostert*
Togniniaceae
P
Esca
Algeria, Iran, Spain
Martin et al. (2011a), ÚrbezTorres et al. (2014)
P. hungaricum Essakhi,
Mugnai, Surico &
Crous*
Togniniaceae
P
Esca
Hungary
Essakhi et al. (2008), BerrafTebbal et al. (2011),
Arzanlou et al. (2014),
Úrbez-Torres et al. (2014),
P. inflatipes W. Gams,
Crous & M.J. Wingf.*
Togniniaceae
P, E
Esca
Chile, Iran, Italy, Spain, USA,
Scheck et al. (1998a, b),
Mugnai et al. (1999),
Whiting et al. (2005),
Mostert et al. (2006),
Gonzalez and Tello (2011),
Mohammadi and
Banihashemi (2012)
P. iranianum L. Mostert,
Gräfenhan, W. Gams &
Crous*
Togniniaceae
P
Esca
Canada, Iran, Italy, South
Africa, Spain
Mostert et al. (2006), Essakhi
et al. (2008), Gramaje et al.
(2009), White et al. (2011),
Mohammadi et al. (2013a),
Sami et al. (2014), ÚrbezTorres et al. (2014)
P. italicum A. Carlucci &
M.L. Raimondo*
Togniniaceae
P
Esca
Italy
Raimondo et al. (2014)
P. krajdenii L. Mostert,
Summerb. & Crous*
Togniniaceae
P
Esca
Canada, Europe, South Africa,
Spain
Mostert et al. (2006), Gramaje
et al. (2011), Úrbez-Torres
et al. (2014)
P. minimum (Tul. & C.
Tul.) D. Gramaje, L.
Mostert & Crous*
Togniniaceae
P
Esca
Argentina, Austria, Australia,
Brazil, Canada, Chile, France,
Germany, Greece, Hungary,
Iran, Israel, Italy, Mexico,
South Africa, Uruguay, USA,
Yugoslavia
Mostert et al. (2006), ÚrbezTorres et al. (2012, 2014),
Baloyi et al. (2013),
Whitelaw-Weckert et al.
(2013)
P. mortoniae Crous & W.
Gams*
Togniniaceae
P
Esca
Iran, New Zealand
Whiting et al. (2005),
Mohammadi and
Banihashemi (2012)
P. occidentale A.B.
Graham, P.R. Johnst. &
B. Weir*
Togniniaceae
P
Esca
New Zealand
Graham et al. (2009),
Arzanlou et al. (2014),
Úrbez-Torres et al. (2014)
P. parasiticum (Ajello,
Georg & C.J.K. Wang)
W. Gams, Crous & M.J.
Wingf.*
P. roseum (J.R.) Úrb.Torr., P. Haag &
O’Gorman*
Togniniaceae
P
Esca
Algeria, Argentina, Australia,
Brazil, Chile, Iran, Peru,
South Africa
Gatica et al. (2001), Dupont
et al. (2002), Berraf-Tebbal
et al. (2011)
Togniniaceae
P
Esca
Canada
da Silva et al. (2017)
P. rubrigenum W. Gams,
Crous & M.J. Wingf.*
Togniniaceae
P
Esca
Argentina, Chile, Croatia,
France, Iran, New Zealand,
South Africa, USA
Dupont et al. (2000),
Kubatova et al. (2004),
Essakhi et al. (2008), Sami
et al. (2014)
123
52
Fungal Diversity (2018) 90:1–84
Table 6 (continued)
Species
Family
Life
mode
Disease caused
Locality
References
P. scolyti L. Mostert,
Summerb. & Crous*
Togniniaceae
P
Esca
France, Italy, South Africa,
Spain, Turkey
Essakhi et al. (2008), Gramaje
et al. (2008), Ozben et al.
(2012), Úrbez-Torres et al.
(2014)
P. sicilianum Essakhi,
Mugnai, Surico &
Crous*
Togniniaceae
P
Esca
Italy, South Africa, Spain
Essakhi et al. (2008), White
et al. (2011), Arzanlou et al.
(2014), Úrbez-Torres et al.
(2014), Gramaje et al.
(2009)
P. subulatum L. Mostert,
Summerb. & Crous*
Togniniaceae
P
Esca
South Africa
Mostert et al. (2006), BerrafTebbal et al. (2011)
P. tuscanicum Essakhi,
Mugnai, Surico &
Crous*
Togniniaceae
P
Esca
Spain
Garcia-Benavides et al. (2013)
P. venezuelense L.
Mostert, Summerb. &
Crous*
Togniniaceae
P
Esca
Algeria, South Africa
Mostert et al. (2006), BerrafTebbal et al. (2011)
P. viticola J. Dupont*
Togniniaceae
P
Esca
France, Germany, Spain
Luque et al. (2009), ÚrbezTorres et al. (2014), Fischer
et al. (2016)
Phaeoacremonium sp.*
Togniniaceae
P, S
Esca
Argentina, China, Iran, South
Africa, Spain
Gatica et al. (2001), Fourie
and Halleen (2002), Halleen
et al. (2003), Gramaje et al.
(2009), White et al. (2011),
Mohammadi and
Banihashemi (2012), This
study
Phaeomoniella
chlamydospora (W.
Gams, Crous, M.J.
Wingf. & Mugnai)
Crous & W. Gams*
Phaeomoniellaceae
P, E
Esca
Argentina, Australia, Brazil,
Bulgaria, Chile, Europe,
France, Iran, Italy, New
Zealand, Slovakia, South
Africa, Spain, Switzerland,
Turkey, Uruguay, USA
Larignon and Dubos (1997),
Crous and Gams (2000),
Karimi et al. (2001),
Cunnington (2003), Halleen
et al. (2003), Whiting et al.
(2005), Kakalikova et al.
(2009), Bobev (2009),
Casieri et al. (2009), Luque
et al. (2009), Smetham et al.
(2010), Gonzalez and Tello
(2011), Correia et al. (2013),
Garcia-Benavides et al.
(2013), Mohammadi et al.
(2013a), Diaz and Latorre
(2014), Akgul et al. (2015)
Phaeotrichoconis
crotalariae (M.A.
Salam & P.N. Rao)
Subram.*
Ascomycota genera
incertae sedis
E
Brazil
Bezerra and De Lima (2012)
Phakopsora ampelopsidis
Dietel & P. Syd.
Phakopsoraceae
P
Rust
Hong Kong, Korea, India,
Taiwan, Thailand
Mundkur (1943), Sawada
(1943), Lu et al. (2000), Cho
and Shin (2004), Lorsuwan
et al. (1984)
P. cronartiiformis Dietel
Phakopsoraceae
P
Rust
India
Mundkur (1943), Padwick
(1946), Watson (1971),
Sarbhoy and Agarwal
(1990)
123
Fungal Diversity (2018) 90:1–84
53
Table 6 (continued)
Species
Family
Life
mode
Disease caused
Locality
References
P. euvitis Y. Ono
Phakopsoraceae
P
Rust
Bangladesh, Brazil, China,
Indonesia, Jamaica, Japan,
Malaysia, North Korea,
Philipines, Thailand,
Thaiwan, USA
Teodoro (1937), Giatgong
(1980), Ono (2000),
Chatasiri and Ono (2008)
P. meliosmae-myrianthae
(Henn. & Shirai) Y.
Ono*
Phakopsoraceae
P
Rust
Japan, Thaiwan
Pota et al. (2015), Ono (2016)
P. montana Y. Ono &
Chatasiri*
Phakopsoraceae
P
Rust
Japan
Pota et al. (2015), Ono (2016)
P. uva Buriticá & J.F.
Hennen*
Phakopsoraceae
P
Rust
Colombia, Costa rica, Cuba,
Guatemala, Mexico, USA,
Venezuela
Buritica and Pardo Cardona
(1996), Pardo Cardona
(1998), Buritica (1999),
Salazar-Yepes et al. (2002)
P. vitis P. Syd.
Phakopsoraceae
P
Rust
Colombia, Costa Rica,
Dominican Republic,
Ecuador, Guatemala,
Indonesia, Japan, Russia,
Taiwan, Trinidad and
Tobago, USA, Venezuela
Arthur (1918), Chardon and
toro (1930), Jackson (1931),
Kern et al. (1934), Baker
and Dale (1951), Berndt
(2004)
Phakopsora sp.
Phakopsoraceae
P
Rust
Costa rica
Berndt (2004)
Phanerochaete viticola
(Schwein.) Parmasto
Phanerochaetaceae
E
Rust
USA
Burdsall (1985)
Phellinidium noxium
(Corner) Bondartseva
& S. Herrera
Hymenochaetaceae
P
Esca
Taiwan
Ann et al. (2002)
Phellinus igniarius (L.)
Quél.
Hymenochaetaceae
P
Esca
Bulgaria
Bobev (2009)
P. resupinatus M. Fisch.,
M. Cloete, L. Mostert
& F. Halleen*
Hymenochaetaceae
P
Esca
Nambia, South Africa
Cloete et al. (2016)
Phellinus sp.*
Hymenochaetaceae
P
Esca
Argentina, Australia, South
Africa, USA
Gatica et al. (2001), Lardner
et al. (2005), Sosnowski
et al. (2007), White et al.
(2011)
Phialophora sp.
Phialosimplex sp.*
Herpotrichiellaceae
Trichocomaceae
E
E, S
Spain
China
Gonzalez and Tello (2011)
Dissanayake et al. (2018),
This study
Phoma confluens Welw.
& Curr.
Didymellaceae
OP
Leaves and
stem lesions
Central Asia
Koshkelova and Frolov (1973)
P. herbarum Westend.*
Didymellaceae
OP
Leaves and
stem lesions
China
Dissanayake et al. (2018)
P. lenticularia Cavara
Didymellaceae
S
Italy
Cavara (1888)
P. medicaginis Malbr. &
Roum.*
Didymellaceae
S
China
This study, Jayawardena et al.
(2018)
P. reniformis Viala &
Ravaz
Didymellaceae
OP
Leaves and
stem lesions
China, Portugal
Phillips and Lucas (1997),
Zhuang (2005)
P. vitis Bonord.
Didymellaceae
OP
Leaves and
stem lesions
Australia, Greece, India, Italy,
USA,
Pantidou (1973), Mathur
(1979), French (1989),
Shivas (1989), Greuter et al.
(1991)
Phoma sp.*
Didymellaceae
P, E,
S
Leaves and
stem lesions
China, Italy, Spain, Switzerland
Casieri et al. (2009), Gonzalez
and Tello (2011), Mondello
et al. (2013), Dissanayake
et al. (2018), This study
123
54
Fungal Diversity (2018) 90:1–84
Table 6 (continued)
Species
Family
Life
mode
Disease caused
Locality
References
Phyllosticta ampelicida
(Engelm.) Aa*
Phyllostictaceae
P, S
Black rot
All over the world
Larter and Martyn (1943),
Mujica and Oehrens (1967),
Alvarez (1976), Mendes
et al. (1998), Dudka et al.
(2004), Kobayashi (2007),
Slippers et al. (2007a, b),
Goos (2010), Wicht et al.
(2012)
P. ampelophila Politis
Phyllostictaceae
P
Black rot
Greece
Pantidou (1973)
P. badamii (Cooke)
Phyllostictaceae
P
Black rot
UK, Ukraine
Watson (1971), Dudka et al.
(2004)
P. microspila Pass.
Phyllostictaceae
P
Black rot
Italy
Watson (1971)
P. muscadinii (Luttr.)
Wulandari
Phyllostictaceae
P
Black rot
USA
Hanlin (1963), Alfieri Jr. et al.
(1984, Kummuang et al.
(1996)
P. pilispora Speschnew
Phyllostictaceae
P
Black rot
China, Japan, Ukraine,
Uzbekistan
Gaponenko (1965), Tai
(1979), Kobayashi (2007),
Dudka et al. (2004)
P. spermoides Peck
Phyllostictaceae
P
Black rot
China, USA
Anonymous (1960), French
(1987, 1989), Bai (2000)
P. turmalis Ellis &
Everh.
Phyllostictaceae
P
Black rot
USA
Cash (1953)
P. vitis-rotundifoliae N.
Zhou & L. Cai*
Phyllostictaceae
P
Black rot
USA
Zhou et al. (2015)
Phytophthora cactorum
(Lebert & Cohn) J.
Schröt.
P. cambivora (Petri)
Buisman
Peronosporaceae
P
Root rot
South Africaa
Oudemans and Coffey (1991),
Erwin and Ribeiro (1996)
Peronosporaceae
P
Root rot
South Africa
Oudemans and Coffey (1991)
P. cinnamomi Rands*
Peronosporaceae
P
Root rot
Australia, New Zealand, South
Africa
P. citricola Sawada
Peronosporaceae
P
Root rot
New Zealand
Gorter (1977), Marais (1980),
Pennycook (1989), Shivas
(1989), Oudemans and
Coffey (1991), Erwin and
Ribeiro (1996), Gadgil
(2005), Blair et al. (2008),
Langrell et al. (2011)
Pennycook (1989), Erwin and
Ribeiro (1996), Gadgil
(2005)
P. cryptogea Pethybr. &
Laff.*
Peronosporaceae
P
Root rot
South Africa
Mills et al. (1991), Erwin and
Ribeiro (1996), Martin et al.
(2014)
P. drechsleri Tucker
Peronosporaceae
P
Root rot
Korea
Cho and Shin (2004)
P. megasperma Drechsler
Peronosporaceae
P
Root rot
Australia, USA
Shivas (1989), Forster and
Coffey (1993)
P. nicotianae Breda de
Haan
Peronosporaceae
P
Root rot
India, South Africa
Erwin and Ribeiro (1996)
P. niederhauseri Z.G.
Abad & J.A. Abad*
Peronosporaceae
P
Root rot
South Africa
Abad et al. (2014)
Phytophthora sp.*
Peronosporaceae
P
Root rot
Australia, Chili, Mexico, USA
Mujica and Oehrens (1967),
Alvarez (1976), French
(1989), Castillo-Pando et al.
(2001), Brasier et al. (2003)
Pilidium concavum
(Desm.) Höhn.
Chaetomellaceae
P
Excoriose and
cane blight
Portugal
Phillips (2000)
123
Fungal Diversity (2018) 90:1–84
55
Table 6 (continued)
Species
Family
Life
mode
Disease caused
Locality
References
P. lythri (Desm.)
Rossman
Chaetomellaceae
P
Excoriose and
cane blight
USA
Greene (1963)
Pionnotes biasolettiana
(Corda) Sacc.
Nectriaceae
E
Japan
Kobayashi (2007)
Plagiostoma devexum
(Desm.) Fuckel*
Gnomoniaceae
E
Europe, USA
Sogonov et al. (2008)
Plasmopara viticola
(Berk. & M.A. Curtis)
Berl. & De Toni
Peronosporaceae
P
All over the world
Doidge (1950), Riley (1960),
Whiteside (1966), Dennis
(1970), Stevenson (1975),
Gorter (1977), Giatgong
(1980), Simonyan (1981),
Mendes et al. (1998),
McKirdy et al. (1999),
Dudka et al. (2004),
Voglmayr et al. (2004),
Gadgil (2005), GarciaBlazquez et al. (2006),
Mulenko et al. (2008),
Thaung (2008b), Bobev
(2009)
Pleospora herbarum
(Pers.) Rabenh.
Pleosporaceae
E
Chile, Libya, Pakistan
Mujica and Oehrens (1967),
El-Buni and Rattan (1981),
Ahmad et al. (1997)
P. penicillus Fuckel
P. phaeocomoides (Sacc.)
G. Winter
Pleosporaceae
Pleosporaceae
S
S
Portugal, Spain
USA
Checa (2004)
Hanlin (1963)
P. vitis Catt.
Pleosporaceae
E
Central Asia, Greece, Italy,
Spain
Unamuno (1941), Koshkelova
and Frolov (1973), Pantidou
(1973), Shoemaker (1992)
P. vitis-viniferae Frolov
Pleosporaceae
E
Central Asia, Russia
Koshkelova and Frolov
(1973), Shoemaker (1992)
Downey
mildew
P. vulgaris Niessl
Pleosporaceae
E
Central Asia
Koshkelova and Frolov (1973)
Pleospora sp.
Pleosporaceae
E
Portugal
Phillips (2000)
Pleurophoma sp.
Lentitheciaceae
P
Excoriose and
cane blight
Portugal
Phillips (2000)
Pleurostoma richardsiae
(Nannfeldt) Réblová &
Jaklitsch*
Pleurostomataceae
P
Trunk disease
Italy, South Africa, Spain
White et al. (2011), Carlucci
et al. (2015), Pintos Varela
et al. (2016)
Pleurotus ostreatus
(Jacq.) P. Kumm.
Pleurotaceae
P
Wood rot
USA
Vail et al. (1995)
Preussia africana Arenal,
Platas & Peláez*
P. intermedia (Auersw.)
S. Ahmad
Sporormiaceae
S
Spain
Garcia-Benavides et al. (2013)
Sporormiaceae
E
Spain
Gonzalez and Tello (2011)
Pseudallescheria sp.*
Microascaceae
S
China
This study
Pseudocamarosporium
propinquum (Sacc.)
Wijayaw., Camporesi
& K.D. Hyde*
Didymospharaceae
S
Italy
This study, Jayawardena et al.
(2018)
P. brachypus (Ellis &
Everh.) X.J. Liu & Y.L.
Guo
Mycosphaerellaceae
P
Leaf spot
USA
Alfieri Jr. et al. (1984
P. daspurensis (A.K. Kar
& M. Manda)
Mycosphaerellaceae
P
Leaf spot
India
Sarbhoy et al. (1971)
123
56
Fungal Diversity (2018) 90:1–84
Table 6 (continued)
Species
Family
Life
mode
Disease caused
Locality
References
Pseudocercospora
riachueli (Speg.)
Deighton
Mycosphaerellaceae
P
Leaf spot
India, Thailand
Kamal (2010), Phengsintham
et al. (2013)
P. vitis (Lév.) Speg.*
Mycosphaerellaceae
P
Leaf spot
Australia, Barbados, Brazil,
Bulgaria, China, France,
Hungary, India, Iowa, Iran,
Italy, Japan, Korea,
Mauritius, Myanmar,
Pakistan, Poland, South
Africa, South Korea, Taiwan,
Tanzania, Thailand, USA,
Zimbabwe
Gilman and Archer (1929),
Wiehe (1948), Riley (1960),
Vasudeva (1963), Whiteside
(1966), Norse (1974),
Deighton (1976), Gorter
(1977), Giatgong (1980),
Thaung (1984), Pons and
Sutton (1988), Cook and
Dubé (1989), Hsieh and Goh
(1990), Ahmad et al. (1997),
Roux et al. (1997), Kim and
Shin (1998), Liu and Guo
(1998), Mendes et al.
(1998), Zhuang (2001),
Dugan et al. (2004),
Kobayashi (2007), Mulenko
et al. (2008), Bobev (2009),
Kamal (2010), Sultan et al.
(2011), Pirnia et al. (2012),
Liang et al. (2016), This
study, Jayawardena et al.
(2018)
Pseudogymnoascus
pannorum (Link)
Minnis & D.L.
Lindner*
Pseudolachnea hispidula
(Schrad.) B. Sutton*
Myxotrichaceae
S
Switzerland
Casieri et al. (2009)
Chaetosphaeriaceae
S
Italy
This study, Jayawardena et al.
(2018)
Pseudopestalotiopsis
camelliae-sinensis F.
Liu & L. Cai*
Sporocadaceae
S
Italy
This study, Jayawardena et al.
(2018)
Pseudopezicula
tetraspora Korf, R.C.
Pearson & W.Y.
Zhuang
Drepanopezizaceae
P
Angular leaf
scorch
USA
Pearson et al. (1988)
P. tracheiphila (Müll.Thurg.) Korf & W.Y.
Zhuang)
Drepanopezizaceae
P
Angular leaf
scorch
Australia, France, Germany,
Hungary, Jordan, Moldova,
Romania, Switzerland,
Tunisia, Turkey, Ukraine,
Yugoslavia
Korf et al. (1986)
Psiloglonium
clavisporum (Seaver) E.
Boehm, C.L. Schoch &
Spatafora
Hysteriaceae
S
USA
Hanlin (1963)
Punctulariopsis
cremeoalbida (M.J.
Larsen & Nakasone)
Ghobad-Nejhad
Punctulariaceae
S
USA
Larsen and Nakasone (1984)
Pyrenochaeta sp.*
Cucurbitariaceae
E
China
Dissanayake et al. (2018)
Pyrenophora
phaeocomes (Rebent.)
Fr.
Pleosporaceae
E
Portugal
Unamuno (1941)
P. phaeocomoides (Berk.
& Broome) Sacc.
Pleosporaceae
E
France, Portugal
Unamuno (1941), Shoemaker
(1992)
123
Fungal Diversity (2018) 90:1–84
57
Table 6 (continued)
Species
Family
Life
mode
Pyrigemmula aurantiaca
D. Magyar & R.
Shoemaker*
Chaetosphaeriaceae
E, S
Pythium acanthicum
Drechsler*
Pythiaceae
P
P. amasculinum Y.N.
Yu*
P. aphanidermatum
(Edson) Fitzp.
Pythiaceae
S
Pythiaceae
P
Disease caused
Locality
References
Hungary
Magyar et al. (2011)
Australia, South Africa
Shivas (1989), McLeod et al.
(2009)
China
This study
Root rot
Australia, South Africa
Cook and Dubé (1989)
Root rot
P. coloratum Vaartaja*
Pythiaceae
P
Root rot
South Africa
McLeod et al. (2009)
P. cryptoirregulare
Garzón, Yánez & G.W.
Moorman*
Pythiaceae
P
Root rot
South Africa
McLeod et al. (2009)
P. debaryanum R. Hesse
Pythiaceae
P
Root rot
Chile, India
Mujica and Vergara (1945)
P. echinulatum V.D.
Matthews*
Pythiaceae
P
Root rot
South Africa
McLeod et al. (2009)
P. helicoides Drechsler*
Pythiaceae
P
Root rot
South Africa
McLeod et al. (2009)
P. heterothallicum W.A.
Campb. & F.F.
Hendrix*
Pythiaceae
P
Root rot
South Africa
McLeod et al. (2009)
P. irregulare Buisman*
Pythiaceae
P
Root rot
Asutralia, South Africa
Cook and Dubé (1989),
Shivas (1989), McLeod
et al. (2009)
P. kunmingense Y.N.
Yu*
Pythiaceae
P
Root rot
South Africa
McLeod et al. (2009)
P. mamillatum Meurs*
Pythiaceae
P
Root rot
Australia, South Africa
Shivas (1989), McLeod et al.
(2009)
P. parasiticum S.
Rajagop. & K. Ramakr.
Pythiaceae
P
Root rot
South Africa
Gorter (1977)
P. paroecandrum
Drechsler*
Pythiaceae
P
Root rot
South Africa
McLeod et al. (2009)
P. periilum Drechsler*
Pythiaceae
P
Root rot
South Africa
McLeod et al. (2009)
P. perplexum H. Kouyeas
& Theoh*
Pythiaceae
P
Root rot
South Africa
McLeod et al. (2009)
P. pyrilobum Vaartaja*
Pythiaceae
P
Root rot
South Africa
McLeod et al. (2009)
P. recalcitrans Belbahri
& E. Moralejo*
Pythiaceae
P
Root rot
South Africa
Moralejo et al. (2008)
P. rostratifingens De
Cock & Lévesque*
Pythiaceae
P
Root rot
South Africa
McLeod et al. (2009)
P. rostratum E.J. Butler
Pythiaceae
P
Root rot
Australia
Cook and Dubé (1989)
P. spinosum Sawada*
Pythiaceae
P
Root rot
Australia, South Africa
Shivas (1989), McLeod et al.
(2009)
P. splendens Hans Braun
Pythiaceae
P
Root rot
Malaysia
Liu (1977)
P. sylvaticum W.A.
Campb. & F.F. Hendrix
P. torulosum Coker & P.
Patt.*
Pythiaceae
P
Root rot
South Africa
Gorter (1977)
Pythiaceae
P
Root rot
South Africa
McLeod et al. (2009)
P. ultimum Trow
Pythiaceae
P
Root rot
Australia, New Zealand, South
Africa
Cook and Dubé (1989),
Shivas (1989), Gadgil
(2005)
P. vanterpoolii V.
Kouyeas & H.
Kouyeas*
Pythiaceae
P
Root rot
South Africa
McLeod et al. (2009)
123
58
Fungal Diversity (2018) 90:1–84
Table 6 (continued)
Species
Family
Life
mode
Disease caused
Locality
References
P. vexans de Bary
Pythiaceae
P
Root rot
Malaysia
Liu (1977)
P. viola Chesters &
Hickman*
Pythiaceae
P
Root rot
South Africa
McLeod et al. (2009)
Pythium sp.*
Pythiaceae
P, S
Root rot
Australia, China, USA
Alfieri Jr. et al. (1984, French
(1989), Castillo-Pando et al.
(2001), This study
Ramularia khandalensis
Patw. & A.K. Pande
Mycosphaerellaceae
P, E
Leaf spot
India
Sarbhoy et al. (1971)
R. mali Videira & Crous*
Mycosphaerellaceae
P, E
Leaf spot
Iran
Bakhshii and Arzanlou (2017)
R. vitis (Richon) U.
Braun
Mycosphaerellaceae
P, E
Leaf spot
Armenia, Australia, Caucasus,
Europe, France
Braun (1998)
Rhabdospora ampelina
(Thüm.) Sacc.
Dothideomycetes
genera incertae
sedis
P
Stem, leaf spot
Japan
Kobayashi (2007)
R. labruscae Gonz. Frag.
Dothideomycetes
genera incertae
sedis
P
Stem, leaf spot
Spain
Gonzalez Fragoso (1917)
R. mueggenburgii
(Pirotta) Sacc.
Dothideomycetes
genera incertae
sedis
P
Stem, leaf spot
Poland
Mulenko et al. (2008)
R. vitis Koshk. & Frolov
Dothideomycetes
genera incertae
sedis
P
Stem, leaf spot
Central Asia
Koshkelova and Frolov (1973)
Rhinocladiella atrovirens
Nannf.
Herpotrichiellaceae
E
Spain
Gonzalez and Tello (2011)
Rhizoctonia solani J.G.
Kühn
Ceratobasidiaceae
P, E
Root rot
South Africa, Spain, USA
Marais (1979), Alfieri Jr. et al.
(1984, Halleen et al. (2003),
Gonzalez and Tello (2011)
Rhizoctonia sp.*
Ceratobasidiaceae
P, E
Root rot
Australia, Chili, Mexico,
Switerzland
Mujica and Vergara (1945),
Alvarez (1976), CastilloPando et al. (2001), Casieri
et al. (2009)
Rhizopus arrhizus A.
Fisch.
Rhizopodaceae
P, E
Bunch rot
USA
French (1987, 1989)
R. oryzae Went & Prins.
Geerl.*
Rhizopodaceae
S
China
This study, Jayawardena et al.
(2018)
R. stolonifer (Ehrenb.)
Vuill.*
Rhizopodaceae
P, E
Bunch rot
Australia, Cuba, Japan,
SouthAfrica, Spain,
Switzerland
Gorter (1977), Urtiaga (1986),
Cook and Dubé (1989),
Witbooi et al. (2000),
Kobayashi (2007), Casieri
et al. (2009), Gonzalez and
Tello (2011)
Rhizopus sp.*
Rhizopodaceae
P, E
Bunch rot
France, Italy, Switzerland
Castillo-Pando et al. (2001),
Casieri et al. (2009),
Mondello et al. (2013)
Rhodosporidium sp.*
Sporidiobolales
genera incertae
sedis
Sporidiobolales
genera incertae
sedis
S
China
This study
S
China
This study
Robillarda vitis Prill. &
Delacr.
Sporocadaceae
E
France
Nag Raj (1993)
Roesleria pallida (Pers.)
Sacc.
Roesleriaceae
P
Japan
Kobayashi (2007)
Rhodotorula sp.*
123
Root rot
Fungal Diversity (2018) 90:1–84
59
Table 6 (continued)
Species
Family
Life
mode
Disease caused
Locality
References
R. subterranea (Weinm.)
Redhead*
Roesleriaceae
P
Root rot
Italy, USA
Kepley et al. (2015)
Rosellinia akulovii L.E.
Petrini
Xylariaceae
S
France
Petrini (2013)
R. amblystoma Berl. & F.
Sacc.
Xylariaceae
S
Portugal
Unamuno (1941)
R. aquila (Fr.) De Not.
Xylariaceae
S
R. necatrix Berl. ex Prill.
Xylariaceae
P
France
Petrini (1992)
Bulgaria, France, Greece, Italy,
Japan, Mexico, Ukraine
Poland
Alvarez (1976), Greuter et al.
(1991), Holevas et al.
(2000), Dudka et al. (2004),
Kobayashi (2007), Bobev
(2009), Petrini (2013)
Mulenko et al. (2008)
R. rosarum Niessl
Xylariaceae
S
Sarocladium strictum
(W. Gams) Summerb.
Hypocreales genera
incertae sedis
E
Spain
Gonzalez and Tello (2011)
Schizophyllum commune
Fr.
Schizothyriaceae
P
White rot on
already dead
parts of
grapevine
trunks
Greece
Zervakis et al. (1998)
Schizothyrium pomi
(Mont.) Arx,
Schizothyriaceae
P
White rot on
already dead
parts of
grapevine
trunks
Japan, USA
Anonymous (1960),
Kobayashi (2007)
Sclerostagonospora sp.
Phaeosphaeriaceae
P
Portugal
Phillips (2000)
Sclerotinia sclerotiorum
(Lib.) de Bary*
Sclerotiniaceae
P, E
Excoriose and
cane blight
Shoot blight
Australia, Chile, Greece, Japan,
Mexico, New Zealand, Spain,
Switzerland, USA
French (1989), Shivas (1989),
Latorre and Guerrero
(2001), Casieri et al. (2009),
Gonzalez and Tello (2011),
Ferrada et al. (2014)
Sclerotium echinatum
Fuckel
Sclerotiniaceae
P
Shoot blight
Poland
Mulenko et al. (2008)
S. rolfsii Sacc.
Sclerotiniaceae
P
Shoot blight
Japan, USA
French (1987, 1989),
Kobayashi (2007)
Sclerotium sp.
Sclerotiniaceae
P
Shoot blight
Thailand
Giatgong (1980)
Scolicotrichum
vitiphyllum
(Speschnew) Karak. &
Vassiljevsky
Ascomycota genera
incertae sedis
P
Shoot blight
Central Asia
Koshkelova and Frolov (1973)
Scopulariopsis sp.*
Microascaceae
S
China
This study
Scytinostroma alutum
Lanq.
Lachnocladiaceae
P, S
Root rot
France
Boidin and Lanquetin (1987)
Seimatosporium botan
Sat. Hatak. & Y.
Harada*
Sporocadaceae
P
Trunk disease
Chile
Diaz et al. (2012)
S. hysterioides (Fuckel)
Brockmann*
Sporocadaceae
P
Trunk disease
Australia, England, France,
Greece, Germany, Italy
Nag Raj (1993), Sergeeva
et al. (2005)
S. lichenicola (Corda)
Shoemaker & E. Müll.
Sporocadaceae
P
Trunk disease
Australia
Cook and Dubé (1989),
Shivas (1989)
S. lonicerae (Cooke)
Shoemaker
Sporocadaceae
P
Trunk disease
Australia
Shivas (1989)
White root rot
123
60
Fungal Diversity (2018) 90:1–84
Table 6 (continued)
Species
Family
Life
mode
Disease caused
Locality
References
S. parasiticum (Dearn. &
House) Shoemaker
Sporocadaceae
P
Trunk disease
Germany, Pakistan
Sutton (1980), Ahmad et al.
(1997)
S. vitis P. Xiao,
Camporesi & K.D.
Hyde*
Sporocadaceae
P, S
Trunk disease
Hungary, Italy
Senanayake et al. (2015),
Váczy (2017), This study,
Jayawardena et al. (2018)
Seiridium cupressi
(Guba) Boesew.
Selenophoma sp.
Sporocadaceae
P
Trunk disease
China
Teng (1996)
Saccotheciaceae
E
Spain
Gonzalez and Tello (2011)
Septobasidium tanakae
(Miyabe) Boedijn &
B.A. Steinm.
Septobasidiaceae
P
Japan
Kobayashi (2007)
Septoria ampelina Berk.
& M.A. Curtis
Mycosphaerellaceae
P
Leaf spot
Bulgaria, Italy, Mexico,
Romania, Ukraine
Radulescu et al. (1973),
Alvarez (1976), Greuter
et al. (1991), Vanev et al.
(1997), Dudka et al. (2004),
Bobev (2009)
S. badhamii Berk. &
Broome
Mycosphaerellaceae
P
Leaf spot
Japan, Romania, UK
Watson (1971), Radulescu
et al. (1973), Kobayashi
(2007)
S. melanopsis Pat.
Mycosphaerellaceae
P
Leaf spot
Brazil, Italy, Kenya, Tunisia,
UK
Nattrass (1961), Watson
(1971)
S. vitis Schulzer
Mycosphaerellaceae
P
Leaf spot
Australia
Priest (2006)
S. vineae Pass.
Mycosphaerellaceae
S
Romania
Watson (1971), Radulescu
et al. (1973)
Septoriella allojunci W.J.
Li, Camporesi, D.J.
Bhat & K.D. Hyde*
Phaeosphaeriaceae
S
China
This study, Jayawardena et al.
(2018)
Simplicillium sp.*
Cordycipitaceae
S
China
This study
Sordaria fimicola
(Roberge ex Desm.)
Ces. & De Not.*
Sordariaceae
S
Switzerland
Casieri et al. (2009)
Sordaria sp.
Sordariaceae
E
Spain
Gonzalez and Tello (2011)
Spencermartinsia
plurivora Abdollahz.,
Javadi & A.J.L.
Phillips*
Botryosphaeriaceae
P
Canker/die
back
Australia, Spain
Pitt et al. (2015)
S. viticola (A.J.L. Phillips
& J. Luque) A.J.L.
Phillips, A. Alves &
Crous*
Botryosphaeriaceae
P
Canker/die
back
Australia, France, South Africa,
Spain, USA
Luque et al. (2005), ÚrbezTorres et al. (2007), de Wet
et al. (2009), Qiu et al.
(2011), Úrbez-Torres
(2011), Diaz et al. (2013),
Pitt et al. (2013, 2015), Li
et al. (2014), Carlucci et al.
(2015), Pavlic-Zupanc et al.
(2015), Valencia et al.
(2015), Comont et al.
(2016), Coutinho et al.
(2017), Lawrence et al.
(2017b)
S. westrale W.M. Pitt,
J.R. Úrbez-Torres &
Trouillas*
Botryosphaeriaceae
P
Canker/die
back
Australia
Pitt et al. (2015)
Spencermartinsia sp.
Botryosphaeriaceae
P
Canker/die
back
Spain
Gonzalez and Tello (2011)
Sphaeropsis ampelos
(Schwein.) Cooke
Botryosphaeriaceae
P
Canker/die
back
China
Teng (1996)
123
Fungal Diversity (2018) 90:1–84
61
Table 6 (continued)
Species
Family
Life
mode
Disease caused
Locality
References
S. peckiana Thüm.
Botryosphaeriaceae
P
Canker/die
back
Italy
Greuter et al. (1991)
S. porosa (Van Niekerk
& Crous) A.J.L.
Phillips & A. Alves
Botryosphaeriaceae
P
Canker/die
back
South Africa
van Niekerk et al.
(2004a, b, 2006), Phillips
et al. (2005), Luque et al.
(2005), de Wet et al. (2009),
Úrbez-Torres (2011)
Sphaeropsis sp.
Botryosphaeriaceae
P
Canker/die
back
Greece
Holevas et al. (2000)
Spiromastix sp.*
Spiromastigaceae
S
China
This study
Spiromyces sp.*
Kickxellaceae
S
China
This study
Sporoschisma ampullula
Sacc.
Chaetosphaeriaceae
S
Yugoslavia
Nag Raj and Kendrick (1975)
Sporocadus rhododendri
(Schwein.) M. Morelet*
Amphisphaeriaceae
P
Cane lesions
Australia
Sergeeva et al. (2005)
Stagonospora bulgarica
Vanev
Phaeosphaeriaceae
P
Leaf spot
Bulgaria
Vanev et al. (1997)
Stachybotrys sp.*
Stachybotryaceae
S
China
This study
Stemphylium viticola
Pass.
Pleosporaceae
E
Poland
Mulenko et al. (2008)
Stemphylium sp.
Pleosporaceae
E
Spain
Gonzalez and Tello (2011)
Stereum hirsutum
(Willd.) Pers.*
Stereaceae
P
Bulgaria, France, Greece, Spain
Larignon and Dubos (1997),
Zervakis et al. (1998),
Bobev (2009), Luque et al.
(2009), Cloete et al. (2015)
Esca
Stereum sp.
Stereaceae
P
Esca
USA
French (1989)
Stigmina esfandiarii Petr.
Mycosphaerellaceae
P
Leaf spot
Iran, Pakistan
Esfandiari and Petrak (1950),
Khan and Kamal (1974)
Strickeria sylvana (Sacc.
& Speg.) Cooke
Sporocadaceae
S
Poland
Mulenko et al. (2008)
S. trabicola (Fuckel) G.
Winter
Sporocadaceae
S
Central Asia
Koshkelova and Frolov (1973)
Stromatoneurospora sp.*
Xylariales genera
incertae sedis
S
China
This study
Talaromyces amestolkiae
N. Yilmaz, Houbraken,
Frisvad & Samson*
Trichocomaceae
S
China
This study, Jayawardena et al.
(2018)
T. pinophilus (Hedgc.)
Samson, N. Yilmaz,
Frisvad & Seifert*
Trichocomaceae
S
China
This study, Jayawardena et al.
(2018)
T. purpureogenum Stoll*
Trichocomaceae
S
China
Talaromyces sp.*
Trichocomaceae
S
China
This study, Jayawardena et al.
(2018)
This study, Jayawardena et al.
(2018)
Terana coerulea (Lam.)
Kuntze
Phanerochaetaceae
P
Wood decay
USA
Campbell et al. (1950), Hanlin
(1966)
Tetracoccosporium sp.
Ascomycota genera
incertae sedis
Ceratobasidiaceae
P
Root stock
disease
South Africa
Halleen et al. (2003)
China
Tai (1979)
Thanatephorus
cucumeris (A.B. Frank)
Donk
S
123
62
Fungal Diversity (2018) 90:1–84
Table 6 (continued)
Species
Family
Life
mode
Thaxteriella pezizula
(Berk. & M.A. Curtis)
Petr.
Tubeufiaceae
S
Thelonectria olida
(Wollenw.) P. Chaverri
& Salgado
Nectriaceae
P
Thielavia sp.
Tilletiopsis minor
Nyland*
Chaetomiaceae
Exobasidiomycetidae
incertae sedis
T. washingtonensis
Nyland
Disease caused
Locality
References
USA
Hanlin (1963)
Uruguay
Abreo et al. (2012)
S
S
China
British Colombia, Canada
This study
Urquhart et al. (1997)
Exobasidiomycetidae
incertae sedis
S
Japan
Urquhart et al. (1997)
Tomentella atramentaria
Rostr.
Thelephoraceae
S
Spain
Hernandez (2004)
T. bryophila (Pers.) M.J.
Larsen
Thelephoraceae
S
Spain
Hernandez (2004)
Black foot
disease
Tomentella sp.*
Thelephoraceae
E
China
Dissanayake et al. (2018)
Torula viticola Allesch.
Torulaceae
E
USA
Saccardo (1878)
Torula sp.
Torulaceae
E
Spain
Gonzalez and Tello (2011)
Toxicocladosporium sp.*
Cladosporiaceae
E
China
Dissanayake et al. (2018)
Trametes zonata (Nees)
Pilát
Polyporaceae
S
New Zealand
Cunningham (1965)
Trichocladium asperum
Harz*
Chaetomiaceae
E, S
Russia, Switzerland
Melnik and Popushoi (1992),
Casieri et al. (2009)
Trichoderma atroviride
P. Karst.*
Hypocreaceae
S
China
This study, Jayawardena et al.
(2018)
T. aureoviride Rifai
Hypocreaceae
E
Spain
Gonzalez and Tello (2011)
T. koningii Oudem.
Hypocreaceae
S
Russia
Melnik and Popushoi (1992)
T. harzianum Rifai*
Hypocreaceae
E, S
China, Spain
Gonzalez and Tello (2011),
This study, Jayawardena
et al. (2018)
T. lixii (Pat.) P. Chaverri*
Hypocreaceae
S
China
This study, Jayawardena et al.
(2018)
T. parapiluliferum (B.S.
Lu, Druzhin. &
Samuels) Jaklitsch &
Voglmayr*
Hypocreaceae
S
Switzerland
Casieri et al. (2009)
Trichoderma sp.*
Hypocreaceae
E
South Africa, Spain,
Switzerland
Fourie and Halleen (2002),
Casieri et al. (2009),
Gonzalez and Tello (2011)
Trichothecium roseum
(Pers.) Link*
Hypocreales genera
incertae sedis
P
Australia, China, Greece, India,
Japan, Korea
Alexopoulos (1940), Tai
(1979), Shivas (1989),
Sharma and Agarwal (1997),
Kobayashi (2007), Oh et al.
(2014), This study
Trullula melanochlora
(Desm.) Höhn.
Leotiomycetes genera
incertae sedis
P
France, Portugal
Phillips (2000)
Truncatella angustata
(Pers.) S. Hughes*
Sporocadaceae
P, E
France, Iran, Portugal, Spain,
Switzerland
Nag Raj (1993), Casieri et al.
(2009), Gonzalez and Tello
(2011), Arzanlou et al.
(2013),
Maharachchikumbura et al.
(2016)
123
Berry rot
Fungal Diversity (2018) 90:1–84
63
Table 6 (continued)
Species
Family
Life
mode
T. pitospora (M.E.A.
Costa & Sousa da
Câmara) Bissett
Sporocadaceae
Typhula viticola (Peck)
Berthier
Disease caused
Locality
References
P
Portugal
Nag Raj (1993)
Typhulaceae
S
USA
Berthier (1976)
Ulocladium sp.
Pleosporaceae
E
South Africa, Spain
Umbelopsis isabellina
(Oudem.) W. Gams*
Mucoraceae
S
Switzerland
Halleen et al. (2003),
Gonzalez and Tello (2011)
Casieri et al. (2009)
Valsaria insitiva (Tode)
Ces. & De Not.
Valsariaceae
P
Portugal, Spain
Phillips (2000), Unamuno
(1941)
Verticillium ahlia Kleb.*
Plectosphaerellaceae
P
China, Japan, USA
French (1989), Kobayashi
(2007), Zhang et al. (2009)
Verticillium sp.
Plectosphaerellaceae
P
Mexico
Alvarez (1976)
Verpa bohemica
(Krombh.) J. Schröt*
Morchellaceae
E
Switzerland
Casieri et al. (2009)
Volutella sp.*
Nectriaceae
S
China
This study
Xeromyces bisporus L.R.
Fraser*
Aspergillaceae
S
Australia
Pettersson et al. (2011)
Xerotus viticola Berk. &
M.A. Curtis
Polyporaceae
S
USA
Berkeley (1872)
Xylaria arbuscula Sacc.
Xylariaceae
S
Taiwan
Ju and Rogers (1999)
Xylaria hypoxylon (L.)
Grev.
Xylariaceae
E
Spain
Gonzalez and Tello (2011)
Xylaria sp.*
Xylariaceae
S
China
This study
Zetiasplozna thuemenii
(Speg.) Nag Raj
Sporocadaceae
S
Italy
Nag Raj (1993)
Life mode—P pathogen, E endophyte, S saprotroph, M mycoparasitic on powdery mildew fungi, OP opportunisitic pathogen and U unknown
*Identification is confirmed by molecular data in the studies. The records are taken from the literatures and thus may not be correct and the same
taxon could be listed more than once. It would be necessary to re -examine all collections if available to confirm their identities. Even the
molecular data may be needed to establish their correct names
but this was shown not to be accurate (Ko et al. 2011). The
most recent studies on fungal pathogens of grapevine have
incorporated multigene analysis to accurately resolve taxa
(Dissanayake et al. 2015; Jayawardena et al. 2015; Yan
et al. 2015; Chethana et al. 2017).
Most previous studies did not address the total community of fungi on Vitis vinifera. Pancher et al. (2012)
carried out an extensive study on endophytes on this host,
showing that how various anthropic and nonanthropic
factors shape microbial communities. There have been
extensive studies on the disease causing agents with more
than 150 taxa known to cause various diseases of grapevine. For example, Colletotrichum species cause grape ripe
rot of Vitis vinifera worldwide (Jayawardena et al. 2016b).
There have however, been no investigation on the saprobes
of grapevines using molecular identification and there has
been no study using mycobiome analysis to reveal saprotrophic communities. The study of saprotrophs is
important, as they not only decay dead leaves and branches, thus beneficial recyclers, but they may also become
pathogens when conditions are suitable.
This study therefore fills this void by establishing the
saprotrophic fungi on Vitis vinifera using both traditional
and culture-independent approaches. In this study we did
not obtain similar results from the two methods. In the
traditional method, 45 species belonging to 30 genera were
identified (Table 2), while in culture-independent method
226 OTUs’ and 72 genera were identified. Even though we
isolated directly from the fruiting bodies, some fungi were
not able to grow on media. Several single spore isolations
were unsuccessful. This may be due to the availability of
nutrient content, pH, temperature, and presence of inhibitors and the time of incubation. The number of isolates
obtained was less than the actual fungal community and
can be misinterpreted (Hugenholtz et al. 1998). These
conditions make it difficult to accurately identify and
123
64
document the vast number of unrecognized taxa (Lücking
and Moncada 2017). For example, in this study the total
identified taxa from the traditional method were 45.
Therefore, to overcome the constraints of traditional
methods, culture-independent techniques are proposed as
an alternative technique (Hoppe et al. 2016).
The aim of environmental sequence nomenclature is to
place names of species of fungi that would otherwise be left
undescribed (Lücking and Moncada 2017). These techniques can provide sequence reads almost 1000 times more
than the traditional DNA sequencing methods (Lücking and
Moncada 2017). Lücking and Moncada (2017) showed that a
formally recognized unnamed lichenicolous basidiomycete
can be considered as a new genus, with seven new species,
although there is no physical type specimens are available.
These authors also suggested that this would allow the
recognition of thousands of species of voucher less taxa
detected through environmental sequencing techniques.
However, there are several constrains to NGS methods. DNA
may not be recovered from all genotypes and the results of
NGS can be biased towards the most abundant organisms at
the time of sampling (Ward et al. 1990). The reason for this is
that the relative abundance (Fig. 5) of microbial species in a
natural habitat is rarely equal. Usually, with a few species
being predominant among a larger group of common species
makes it difficult to identify the species that are actually
present. NGS are mainly based on analysis of ITS regions
(Schoch et al. 2012). However, due to the high variability of
ITS regions (ITS1 and ITS2), reliable sequence alignments
are difficult to obtain for some fungal taxa. Therefore, this
method is not reliable for species level identification. The
identification levels are usually reported at the genus level or
Fig. 5 Relative abundance of
the top 10% phylum from
different samples of the
cultivars Carbanate Gernischet
and Red Globe of Vitis vinifera
123
Fungal Diversity (2018) 90:1–84
even higher taxonomic levels, such as family or order (Purahong et al. 2018). Another constraint of NGS is that the
correspondence of OTU with species can be unreliable.
OTUs are defined based on the similarity threshold, usually
with a 97% (Sneath and Sokal 1973). However, some species
have genes that are 97% similar, which will result in merged
OTUs containing multiple species. In the same way, a single
species may have paralogs that are \ 97% similar, causing
the species to be split across two or more species. Some
identified clusters, even when a majority, may be false, due to
the artifacts including reading errors and chimeras (Sneath
and Sokal 1973). Assessing species richness and diversity of
a microbial community using culture-independent method
(rarefaction curves), suggests that OTUs are observations of
organisms with ‘negligible error’. Also, it suggests that the
number of reads correlates well with the total number of
individuals present in the community. However, if the
majority of OTUs are experimental artifacts, the traditional
species richness estimations cannot be applied. The measures between sample variations will tend to reflect differences in artifact frequencies rather than biological
differences (Sokal and Sneath 1963).
Artifacts can be occurred due to several reasons. PCR
amplification steps can be affected by preferentially/differentially that can hinder the detection of some genotypes
when analysing bulk DNA extracts from a substrate
(Kanagawa 2003). Primer mismatches, a lower rate of
primer hybridization, occurrence of heteroduplexes and
chimeric amplicons can generate additional signals that do
not correspond to the genotypes in the same samples
(Suzuki and Giovannoni 1996; Kanagawa 2003). Also, the
Fungal Diversity (2018) 90:1–84
analysis of fungal rRNA genes limits identification to the
genus or family level (Anderson and Cairney 2004).
Dissanayake et al. (2018) in her study using paired-end
Illumina sequencing with 55, 822 high quality sequences
per endophyte sample (saturated rarefaction curves for all
samples) revealed 59 OTUs (the majority containing genera level identification) that were similar to genera revealed
by the traditional method (28 species).
Traditional versus culture-independent methods:
can matching of these two approaches enable us
to identify correct fungal taxonomic information
at genus and species levels?
In this study, taxa (OTUs) of Aspergillus, Botrytis, Cladosporium, Clonostachys, Fusarium, Penicillium, Phoma and
Talaromyces were identified using both traditional and culture-independent approaches. Some fast growing fungi may
be dominant in the culture plates, even though in the natural
habitat they may be minorities. Many hyphomycetes tend to
grow faster than the other groups of fungi. So, they may suppress the growth of other important, dominant fungi. The fast
growing fungi (hyphomycetes) identified in the traditional
method such as Mucor and Rhizopus were not recognized in
the culture-independent method. The majority of the genera
identified in the traditional method are phytopathogens, while
in the culture-independent method the majority are saprotrophs. In the traditional method using both morphological and
molecular approaches, we were able to identify many taxa to
species level, although in six cases the identification is only up
to the genus level due to lack of data. We have generated a
phytogenetic tree for the genus Colletotrichum using the
strains identified in the traditional approach as well as the OTU
identified in the culture-independent method. OTU-234, was
identified as Glomerellaceae sp. in the culture-independent
approach. The blastn result of OTU-234 in NCBI shows 100%
similarity to many strains of C. gloeosporioides. Two-hundred
and fifteen basepairs of OTU-234 were used in the alignment
(Supplementary Fig. S6). In the phylogenetic tree constructed
using the ex-type strains of gloeosporioides complex and the
truncatum complex, OTU-234 cluster within the truncatum
complex, closely to C. curcumae (Supplementary Fig. S7).
This example also provides evidence that the NGS sequences
is not reliable to identify an organism to the species level.
However, in the culture-independent technique we were able
to identify 90 out of 226 OTUs to species level, and the rest
were identified to genera or family level. These may not be
correctly identified as in general NGS fungal taxa identification may be only accurate to the genus level (Purahong et al.
2018), which suggests that the sequence data from the cultureindependent approach is inadequate to accurately identify
species. The overlap between the two methods in identifying
the taxa to the species level is negligible.
65
Matching between the traditional and culture-independent data allows us to have a better understanding concerning
the functional information of the fungal OTUs resulting from
culture-independent methods. Next generation sequencing
often results in sequences that are associated with taxa,
which have not been reported in previous studies (Tejesvi
et al. 2010; Ko et al. 2011; Taylor et al. 2016). However, as
most of these OTUs are identified to genus or family level, it
makes it difficult to relate whether these are actually correctly identified and whether the use of this method is
important. In the preparation of the checklist of fungi on Vitis
species, the authors had to eliminate most of the taxa that
were identified using NGS, as those data can be unreliable. In
our study, we compared the sequence similarity between the
two cultivars using a 90% similarity of ITS1 sequence data,
followed by a manual BLAST based identification of the
respective OTUs. We considered the ITS similarity at
98–99% as the same species (Garnica et al. 2016; Jeewon and
Hyde 2016). In this criterion, identification of genera can be
bias/difficult as some of the data in databases have mistakes
or they may be inaccurate. The increase of the ITS similarity
to 99–100% can give us better and reliable identification of
the species. However, ITS sequence data alone will not be
able to identify the complexes genera such as Colletotrichum
and Diaporthe to their species level. For a better resolution of
these genera protein coding gene regions are required.
Can direct matching between traditional
and culture-independent methods help
to identify the rare taxa?
Our results show that some singletons, which were usually
removed as artifacts or errors of the NGS may actually be
real OTUs. In this study, we found two OTUs (Botryospaeria OTU-178 and Ascomycota OTU-213) as singletons
and removed them from the analysis. However, with direct
matching, we found that these OTUs are Botryospaeria
dothidea and Coniella vitis. Therefore, we can assume that
not all the singletons are artifacts and matching between
traditional and culture-independent methods can help to
identify the real rare taxa in the fungal community.
Potential effect of grape cultivars (table grape
(Red Globe) and wine grape (Carbanate
Gernischet) on fungal saprotrophic community
composition and richness
Another aspect of this study was to study whether there is
any difference in the fungal communities based on cultivars. In the present study, traditional and culture-independent approaches allows the identification of potential roles
of the saprotrophs in the two grapevine cultivars. In this
study we identified more than 10 main and important
123
66
fungal pathogens of grapevine using both methods. With
the evaluation of both community composition and community diversity we were able to identify that the fungal
communities of the two grape cultivars appear to be different. Alternaria vitis, Albifrimbria viridis, Bipolaris
maydis, Botryosphaeria dothidea, Botrytis cinerea, Colletotrichum hebeinse, C. truncatum, C. viniferum, Didymella pomorum, Dothiorella sarmentorum, Epiccocum
nigrum, Fusarium sp., Mucor circinelloides, Paraphoma
chrysanthemicola,
Neopestalotiopsis
clavispora,
Stagonosporopsis sp.1, Minimedusa sp., Peniophora sp.,
Penicillium brevicompactum and P. citrinum were recorded only from Red Globe cultivar while Albifimbria verrucaria, Neopestalotiopsis vitis, Pythium amasculinum,
Stagonosporopsis sp.2, Trichoderma lixii and Septoriella
allojunci were recorded from Carbanate Gernischet cultivar in the traditional method. In the culture-independent
approach, Acremonium chrysogenum (OTU-195), Apodus
sp. (OTU-235), Ascomycota (OTU-80, 99, 182, 222, 253),
Aspergillus sp. (OTU-116, 199), Candida mucifera (OTU227), Cylindrocarpon sp. (OTU-171), Dactylellina phymatopaga (OTU-58), Davidiella tassiana (OTU-86),
Deroxomyces sp. (OTU-225), Fungal (OTU-245, 254),
Fusarium cf. dimerum (OTU-162), Helotiales (OTU-91),
Hypocreales (OTU-65), Kernia nitida (OTU-184), Kernia
pachypleura (OTU-211), Lecanicilium dimorphum (OTU101), Lentinus squarrosulus (OTU-249), Lophiostoma sp.
(OTU-142), Microascales (OTU-138), Metarhizium pinghaense (OTU-210), Myceliophthora fergusii (OTU-198),
Myrothecium sp. (OTU-238), Nectriaceae (OTU-97, 194),
Papulospora equi (OTU-148), Phialosimplex caninus
(OTU-187), Psathyrellaceae (OTU-145), Pseudallescheria
angusta (OTU-183), Pyronemataceae (OTU-237), Remersonia sp. (OTU 108), Sordariomycetes (OTU-128), Sordariales (OTU-196, 200, 214), Xylaria sp. (OTU-159) were
found only in association with the Red Globe cultivar while
Acremonium sp. (OTU-188), Apllosporella yalgorensis
(OTU-85), Arachnomyces kanei (OTU-170), Aspergillus
melleus (OTU-143), Aspergillus wentii (OTU-175), Cadophora luteo-olivaceae (OTU-146), Ceratobasidiaceae
(OTU-219), Chaetomium carinthiacum (OTU-177), Chysisporium lobatum (OTU-150), Cladosporium grevilleae
(OTU-121), Dothideomycetes (OTU-140), Eurotiales
(OTU-76), Fungal (OTU-82, 104, 165), Gymnascella
aurantiaca (OTU-151), Hansfodia sp. (OTU-232),
Hypocreales (OTU-49, 92, 202), Lasiophaeriaceae (OTU189), Leptosphaeria sp. (OTU-205), Magnoporthaceae
(OTU- 141, 149), Microascales (OTU-114), Microascus sp.
(OTU-185), Microdochium sp. (OTU-225), Nectriaceae
(OTU-218), Penicillium ilerdanum (OTU-163), Penicillium neocrassum (OTU-168), Podospora communis (OTU190), Scopulariopsis sp. (OTU-164), Sordariales (OTU133), Spiromastix princeps (OTU-139), Thielavia basicola
123
Fungal Diversity (2018) 90:1–84
(OTU-155), Trichomaceae (OTU-156, 166) were recorded
on from Carbanate Gernischet cultivar.
The difference of the two fungal communities can be
due to the geographic variation of the cultivars. This can be
a result from the interactions with specific V. vinifera
varieties and its soil and climatic conditions (Bokulich
et al. 2014). Red Globe cultivar was collected in Beijing,
which is a region in North of China and Carbanate Gernischet cultivar was collected from Yunnan which is in the
southern part of the country. The difference between the
fungal communities in regions may be a function of a
neutral process, where these different communities established by chance and lack of species dispersal allows these
communities to persist (Martiny et al. 2006). This difference can also be due to the Baas Becking hypothesis,
which states that there is no limit to the range of species but
that selection sorts these species and defines community
composition and diversity in any one area (Hanson et al.
2012). Climate can also co-relates with differences in
fungal communities in China, as one moves North up in
China, the climate becomes increasingly cold and dry so
the pattern of lower fungal species richness in the northern
most regions hints that selection might have a role in
determining these patterns.
Plant pathogens and endophytes
in the saprotrophic fungal community
Species richness and distribution patterns of saprotrophic
fungi in a vineyard can provide important insights into the
roles of each fungal group for the stability and functioning
of its respective ecosystem (Kubartova et al. 2012). However, knowledge of saprotrophic fungi associated with
grapevine is very much limited. In this study, we identified
17 primary and six species of secondary pathogens of
grapevine as saprobes using the traditional method, while
27 OTUs were identified as both primary and secondary
pathogens from dead material of Vitis vinifera in the culture-independent method.
Species of Alternaria are responsible in causing berry
rots, raisin molds and rots as well as pedicel and rachis
diseases (Barbe and Hewitt 1965; Gonzalez and Tello
2011; Tao et al. 2014, Ariyawansa et al. 2015) and also
considered as wound and secondary invaders. Alternaria
alternata and A. vitis were isolated in this study. Aspergillus is a causal agent of berry rots as well as a wound and
secondary invader (Hewitt 2015). In our study A. aculeatus
and A. niger were recorded using the traditional method,
while A. aculeatus was also recorded from culture-independent method. Botryosphaerious taxa are well-known to
be associated with grapevine canker and die back (ÚrbezTorres et al. 2012, 2013a, b). In our study we identified
Botryosphaeria dothidea and Dothiorella sarmentorum as
Fungal Diversity (2018) 90:1–84
saprotrophs using traditional methodology. Lasiodiplodia
was recorded in the culture-independent method.
Botrytis is another genus that we obtained in both traditional and independent approaches. Botrytis cinerea is a
pathogen of grapevine causing Botrytis bunch rot and
blight all over the world (Fournier et al. 2013; Hyde et al.
2014; Javed et al. 2017). Cladosporium was also recorded
in both approaches. Species of this genus cause minor
foliage diseases of grapevine, as well as bunch rots (Bensch
et al. 2015). Clonostachys is another genus recorded in
both approaches. Clonostachys rosea is known to cause
root rot of grapevine in Switzerland (Casieri et al. 2009).
Colletotrichum hebeiense, C. truncatum and C. viniferum
were recorded in the traditional method. Species of this
genus cause grape ripe rot affecting the quality and production of grapevine (Yan et al. 2015). Diaporthe eres is
another pathogen of grapevine causing die back (Lawrence
et al. 2015; Baumgartner et al. 2013; Cinelli et al. 2016;
Fischer et al. 2016; Bastide et al. 2017), which was
recorded via the traditional methodology as well as via the
culture-independent approach.
Species of Fusarium cause wilt disease of grapevine
(Castillo-Pando et al. 2001; Gonzalez and Tello 2011).
This genus was recorded in both approaches. Neopestalotiopsis vitis recorded from traditional method is a pathogen
causing fruit rot, die back and leaf spots of grapevine
(Jayawardena et al. 2015, 2016a). Coniella vitis is a
pathogen causing white rot of grapes, identified using traditional methods (Chethana et al. 2017). Species of Penicillium are wound and secondary pathogens of grapevines
causing bunch rot (Kim et al. 2007). Rhizopus oryzae is
another wound and secondary pathogen causing bunch rots
of grapevines (Hewitt 2015).
Several genera were identified only in the culture-independent method. Aplosporella is known to cause lesions on
grapevine stems in China (Tai 1979). Claviceps is known to be
a pathogen on grasses and cereals, but has not been recorded as
a pathogen of grapevine (Mey et al. 2002). Therefore, this
study provides the first record of this genus on V. vinifera.
Cylindrocarpon species are known to cause the black foot
disease of grapevine (Abreo et al. 2010, 2012; Mohammadi
et al. 2013a, b). Devriesia is a facultative pathogen, but there
are no records of this species on V. vinifera (Seifert et al.
2004). Therefore, this study provides the first record of this
genus on V. vinifera. Species of Leptosphaeria has been
reported as endophytes and saprotrophs of grapevine (Crane
and Shearer 1991). However, some species of this genus can
be pathogenic to some economically important crops (Fitt
et al. 2006). Monographella is a known leaf pathogen on rice,
barley, maize and wheat (Daamen et al. 1991; Hock et al.
1992; Tatagiba et al. 2015). However, there are no records of
species of this genus associated with grapevine. Therefore,
this study provides the first record of Monographella
67
associated with grapevine. Species of Phaeoacremonium are
causal agents of Esca disease around the world (Garcia-Benavides et al. 2013). Species of Trichothecium are known to
cause berry rot of grapevine, but this is not considered as a
major pathogen on grapevine (Oh et al. 2014).
Even though genus Volutella is a facultative pathogen
causing leaf spot and cankers (Henricot et al. 2000; Shi and
Hsiang 2014), there is no record of this genus occurring on
grapevine. Therefore, this study provides the first record of
Volutella associated with V. vinifera as a saprotroph.
Among the 45 identified saprotrophic taxa, 17 are well
known pathogens of Vitis vinifera causing severe yield as
well as economic losses to viticulture worldwide (Table 2).
Six secondary pathogens of were also identified in this
study. Most of the pathogens tend to survive or overwinter
on dead plant material as saprotrophs and act as the primary inoculums once the conditions are favourable (Armijo et al. 2016).
Many studies have shown that most pathogenic fungi
can survive unsuitable conditions, such as cold during the
winter, by changing their life mode to saprotrophs, and
become active pathogens again once the conditions are
suitable. Therefore, dead plant materials are the potential
primary inocula for plant pathogens in vineyards. In order
to avoid this problem, vineyards must be kept clean. If
there are any dead grapevines they must be removed and if
possible should be burned. This will reduce the pathogenic
fungi from year to year.
Checklist of fungi on Vitis
Nine-hundred and five micro- and macro- fungal taxa
reported on Vitis species are listed in this study. This is an
updated worldwide checklist of fungi on Vitis. These taxa
are distributed in 156 families and 343 genera. For each
species, family, life mode, diseases caused and the known
locality as well as references are provided.
Acknowledgements This work was financially supported by Beijing
Talent Programm for Jiye Yan, CARS-29 and JNKYT201605.
Open Access This article is distributed under the terms of the
Creative Commons Attribution 4.0 International License (http://crea
tivecommons.org/licenses/by/4.0/), which permits unrestricted use,
distribution, and reproduction in any medium, provided you give
appropriate credit to the original author(s) and the source, provide a
link to the Creative Commons license, and indicate if changes were
made.
References
Abad ZG, Abad JA, Cacciola SO, Pane A, Faedda R, Moralejo E,
Perez-Sierra A, Abad-Campos P, Alvarez-Bernaola LA, Bakonyi
J, Jozsa A, Herrero ML, Burgess TI, Cunnington JH, Smith IW,
Balci Y, Blomquist C, Henricot B, Denton G, Spies C, McLeod
123
68
A, Belbahri L, Cooke D, Kageyama K, Uematsu S, Kurbetli I,
Degirmenci K (2014) Phytophthora niederhauserii sp. nov., a
polyphagous species associated with ornamentals, fruit trees and
native plants in 13 countries. Mycologia 106:431–447
Abreo E, Martinez S, Bettucci L, Lupo S (2010) Morphological and
molecular characterization of Campylocarpon and Cylindrocarpon spp. associated with black foot disease of grapevines in
Uruguay. Australas Plant Pathol 39:446–452
Abreo E, Lupo S, Bettucci L (2012) Fungal community of grapevine
trunk diseases: a continuum of symptoms? Sydowia 64:1–12
Agusti-Brisach C, Pérez-Sierra A, Garcı́a-Figueres F, Montón C,
Armengol J (2011) First report of dampingoff caused by
Cylindrocarpon pauciseptatum on Pinus radiata in Spain. Plant
Dis 95:874
Agusti-Brisach C, Alaniz S, Gramaje D, Perez-Sierra A, Armengol J
(2012) First report of Cylindrocladiella parva and Cylindrocladiella peruviana associated with black-foot disease of grapevine in Spain. Plant Dis 96:1381
Agusti-Brisach C, Cabral A, Gonzalez-Dominguez E, Perez-Sierra A,
Leon M, Abad-Campos P, Garcia-Jimenez J, Oliveira H,
Armengol J (2016) Characterization of Cylindrodendrum,
Dactylonectria and Ilyonectria isolates associated with loquat
decline in Spain, with description of Cylindrodendrum alicantinum sp. nov. Eur J Plant Pathol 145:103–118
Ahmad S (1969) Fungi of West Pakistan. Biol Soc Pak Monogr
5(Suppl. 1):1–110
Ahmad S (1978) Ascomycetes of Pakistan, Part II. Biol Soc Pak
Monogr 8:1–144
Ahmad S, Iqbal SH, Khalid AN (1997) Fungi of Pakistan. Sultan
Ahmad Mycological Society of Pakistan, Lahore
Akgul DS, Savas NG, Eskalen A (2014a) First report of wood canker
caused by Botryosphaeria dothidea, Diplodia seriata, Neofusicoccum parvum, and Lasiodiplodia theobromae on grapevine in
Turkey. Plant Dis 98:568
Akgul DS, Savas NG, Onder S, Ozben S, Kaymak S (2014b) First
report of Campylocarpon fasciculare causing black foot disease
of grapevine in Turkey. Plant Dis 98:1277
Akgul DS, Gungor Savas N, Teker T, Keykubat B, Mayorquin JS,
Eskalen A (2015) Fungal trunk pathogens of Sultana seedless
vineyards in Aegean region of Turkey. Phytopathol Mediterr
54:380–393
Alaniz S, Leon M, Vicent A, Garcia-Jimenez J, Abad-Campos P,
Armengol J (2007) Characterization of Cylindrocarpon species
associated with black foot disease of grapevine in Spain. Plant
Dis 91:1187–1193
Alaniz S, Armengol J, Leon M, Garcia-Jimenez J, Abad-Campos P
(2009) Analysis of genetic and virulence diversity of Cylindrocarpon liriodendra and C. macrodidymum associated with black
foot disease of grapevine. Mycol Res 113:16–23
Alexopoulos CJ (1940) Some fungi from Greece. Mycologia
32:336–358
Alfieri Jr SA, Langdon KR, Wehlburg C, Kimbrough JW (1984)
Index of plant diseases in Florida (revised). Florida Department
of Agriculture and Consumer Services, Division of Plant
Industry Bulletin, vol 11, pp 1–389
Alfieri SA Jr, Langdon KR, Kimbrough JW, El-Gholl NE, Wehlburg
C (1994) Diseases and disorders of plants in Florida. Florida
Department of Agriculture and Consumer Services, Tallahassee
Al-Saadoon AH, Ameen MKM, Hameed MA, Al-Badran A, Ali Z
(2012) First report of grapevine dieback caused by Lasiodiplodia
theobromae and Neoscytalidium dimidiatum in Basrah, Southern
Iraq. Afr J Biotechnol 11:16165–16171
Alvarez MG (1976) Primer catalogo de enfermedades de plantas
Mexicanas. Fitofilo 71:1–169
Alves A, Linaldeddu BT, Deidda A, Scanu B, Phillips AJL (2014)
The complex of Diplodia species associated with Fraxinus and
123
Fungal Diversity (2018) 90:1–84
some other woody hosts in Italy and Portugal. Fungal Divers
67:143–156
Amrani L, Corio-Costet M-F (2006) A single nucleotide polymorphism in the ß-tubulin gene distinguishing two genotypes of
Erysiphe necator expressing different symptoms on grapevine.
Plant Pathol 55:505–512
Anderson IC, Cairney JW (2004) Diversity and ecology of soil fungal
communities: increased understanding through the application of
molecular techniques. Environ microbiol 6:769–779
Ann PJ, Chang T-T, Ko W-H (2002) Phellinus noxius brown root rot
of fruit and ornamental trees in Taiwan. Plant Dis 86:820–826
Anonymous (1960) Index of plant diseases in the United States.
U.S.D.A. Agricultural Handbook 165:1–531
Anonymous (1979) List of plant diseases in Taiwan. The Plant
Protection Society of The Republic of China, Taichung
Ariyawansa HA, Thambugala KM, Manamgoda DS, Jayawardena R,
Camporesi E, Boonmee S, Wanasinghe DN, Phookamsak R,
Hongsanan S, Singtripop C, Chukeatirote E (2015) Towards a
natural classification and backbone tree for Pleosporaceae.
Fungal Divers 71:85–139
Armijo G, Schlechter R, Agurto M, Muñoz D, Nuñez C, ArceJohnson P (2016) Grapevine pathogenic microorganisms: understanding infection strategies and host response scenarios. Front
Plant Sci 7:382
Arnold GRW (1986) Lista de Hongos Fitopatogenos de Cuba.
Ministerio de Cultura Editorial Cientifico-Tecnica, Habana
Arthur JC (1918) Uredinales of Guatemala based on collections by
E.W.D. Holway. I. Introduction. Coleosporiaceae and Uredinaceae. Am J Bot 5:325–336
Arzanlou M, Moshari S, Bakhshi M, Khodaie S (2012) Botryosphaeria dothidea associated with grapevine decline disease in
Iran. Australas Plant Dis Notes 7:197–200
Arzanlou M, Narmani A, Moshari S, Khodaei S, Babai-Ahari A
(2013) Truncatella angustata associated with grapevine trunk
disease in Northern Iran. Arch Phytopathol Pflanzenschutz
46:1168–1181
Arzanlou M, Narmani A, Khodaei S, Moshari S (2014) Pome and
stone fruit trees as possible resevoir hosts for Phaeoacremonium
spp., the causal agents of grapevine esca disease, in Iran. Arch
Phytopathol Pflanzenschutz 47:717–727
Auger J, Esterio M, Ricke G, Perez I (2004a) Black dead arm and
basal canker of Vitis vinifera cv. red globe cause by Botryosphaeria obtuse in Chile. Plant Dis 88:1286
Auger J, Esterio M, Perez I, Gubler WD, Eskalen A (2004b) First
report of Phaeomoniella chlamydospora on Vitis vinifera and
French American hybrids in Chile. Plant Dis 88:1285
Bai J-K (ed) (2000) Flora Fungorum Sinicorum. Sphaeropsidales,
Phoma, Phyllosticta, vol 15. Science Press, Beijing
Baker RED, Dale WT (1951) Fungi of Trinidad and Tobago. Mycol
Pap 33:1–123
Bakhshi M, Arzanlou M (2017) Multigene phylogeny reveals a new
species and novel records and hosts in the genus Ramularia from
Iran. Mycol Progr 16:703–712
Bakhshi M, Arzanlou M, Babai-Ahari A (2012) Comprehensive
check list of Cercosporoid fungi from Iran. Plant Pathol Quar
2:44–55
Balmas V, Scherm B, Ghignone S, Salem AOM, Cacciola SO,
Migheli Q (2005) Characterisation of Phoma tracheiphila by
RAPD-PCR, microsatellite-primed PCR and ITS rDNA sequencing and development of specific primers for in planta PCR
detection. Eur J Plant Pathol 111:235–247
Baloyi MA, Halleen F, Mostert L, Eskalen A (2013) First report of
Togninia minima perithecia on esca- and Petri-diseased grapevines in South Africa. Plant Dis 97:1247
Barbe GD, Hewitt WB (1965) Principal fungus in summer bunch rot
of grapes. Phytopathology 55:815
Fungal Diversity (2018) 90:1–84
Baroncelli R, Sreenivasaprasad S, Lane CR, Thon MR, Sukno SA
(2014) First report of Colletotrichum acutatum sensu lato
(Colletotrichum godetiae) causing anthracnose on grapevine
(Vitis vinifera) in the United Kingdom. New Dis Rep 29:26
Barr ME (1990) Some dictyosporous genera and species of Pleosporales in North America. N Y Bot Gard 62:1–92
Barr ME (1992) Notes on the Lophiostomataceae (Pleosporales).
Mycotaxon 45:191–221
Baskarathevan J, Jaspers MV, Jones EE, Ridgway HJ (2008)
Distribution of Botryosphaeria species causing grapevine dieback and decline in New Zealand vineyards. NZ Plant Protect
61:392
Baskarathevan J, Jaspers MV, Ridgway HJ, Eirian JE (2012)
Incidence and distribution of Botryosphaeriaceous species in
New Zealand vineyards. Eur J Plant Pathol 132:549–560
Bastide F, Serandat I, Gombert J, Laurent E, Morel E, Kolopp J,
Guillermin PL, Hamon B, Simoneau P, Berruyer R, Poupard P
(2017) Characterization of fungal pathogens (Diaporthe angelicae and D. eres) responsible for umbel browning and stem
necrosis on carrot in France. Plant Pathol 66:239–253
Batista AC, Ciferri R (1962) The Chaetothyriales. Sydowia 3:1–129
Batra LR (1973) Nematosporaceae (Hemiascomycetidae): taxonomy,
pathogenicity, distribution, and vector relationships. U.S.D.A.
Agric Res Serv Tech Bull 1469:1–71
Baumgartner K, Fujiyoshia PT, Travadon R, Castlebury LA, Wilcox
WF, Rolshausen PE (2013) Characterization of species of
Diaporthe from wood cankers of grape in eastern North
American vineyards. Plant Dis 97:912–920
Beale RE, Pitt D (1990) Biological and integrated control of Fusarium
basal rot of Narcissus using Minimedusa polyspora and other
micro-organisms. Plant Pathol 39:477–488
Bechet M, Sapta-Forda A (1981) Investigation on the growth,
development and control of Alternaria vitis Cav., the pathogen
of alternariosis of grapevine. Romania Univ’ersitatea BabesBloya, pp 147–156
Begon M, Harper JL, Townsend CR (1993) Ecology: Individuals,
Population and Communities, 3rd edn. Blackwell Science,
Boston
Begoude AD, Slippers B, Wingfeld MJ, Roux J (2010)
Botryosphaeriaceae associated with Terminalia catappa in
Cameroon, South Africa and Madagascar. Mycol Progr
9:101–123
Benavides PG, Zamorano PM, Ocete CA, Maistrello L, Ocete R
(2013) Biodiversity of pathogenic wood fungi isolated from
Xylotrechus arvicola (Olivier) galleries in vine shoots. OENO
One 47:73–81
Bendezu-Euribe MV, Alvarez LA (2012) The perfect stage of
powdery mildew of grapevine caused by Erysiphe necator found
in Peru. Plant Dis 96:768
Benjamin CR, Slot A (1969) Fungi of Haiti. Sydowia 23:125–163
Bensch K, Groenewald JZ, Braun U, Dijksterhuis J, de Jesús Y-MM,
Crous PW (2015) Common but different: the expanding realm of
Cladosporium. Stud Mycol 82:23–74
Berkeley MJ (1872) Notices of North American fungi. Grevillea
1:33–39
Berndt R (2004) A checklist of Costa Rican rust fungi. In: Agerer R,
Piepenbring M, Blanz P (eds) Frontiers in Basidiomycete
Mycology. IHW-Verlag, Berlin
Berraf-Tebbal A, Bouznad Z, Santos JM, Coelho MA, Peros J-P,
Phillips AJL (2011) Phaeoacremonium species associated with
Eutypa dieback and esca of grapevines in Algeria. Phytopathol
Mediterr 50:S86–S97
Berraf-Tebbal A, Guereiro MA, Phillips AJL (2014) Phylogeny of
Neofusicoccum species associated with grapevine trunk disease
in Algeria, with decription of Neofusicoccum algeriense sp. nov.
Phytopathol Mediterr 53:416–427
69
Berthier J (1976) Monographie des Typhula, Pistillaria et des genres
voisins. Bull Soc Linn Lyon 45:1–213
Bezerra JL, De Lima TEF (2012) Phaeotrichoconis crotalariae,
endophytic on Vitis labrusca, in Brazil. Mycotaxon 120:291–294
Billones RG, Ridgway HJ, Jones EE, Jaspers MV (2010) First report
of Neofusicoccum macroclavatum as a canker pathogen of
grapevine in New Zealand. Plant Dis 94:1504
Blair JE, Coffey MD, Park SY, Geiser DM, Kang S (2008) A multilocus phylogeny for Phytophthora utilizing markers derived
from complete genome sequences. Fungal Genet Biol
45:266–277
Bobev S (2009) Reference guide for the diseases of cultivated plants.
http://nt.ars-grin.gov/fungaldatabases
Boesewinkel HJ (1982) A list of 142 new plant disease recordings
from New Zealand and short notes on three diseases. Australas
Plant Pathol 11:40–43
Boidin J, Lanquetin P (1987) Le genre Scytinostroma Donk (basidiomycetes, Lachnocladiaceae). Biblioth Mycol 114:1–130
Bokulich NA, Subramanian S, Faith JJ, Gevers D, Gordon JI, Knight
R, Mills DA, Caporaso JG (2013) Quality-filtering vastly
improves diversity estimates from Illumina amplicon sequencing. Nat Methods 10:57–59
Bokulich NA, Thorngate JH, Richardson PM, Millis DA (2014)
Microbial biogeography of wine grapes is conditioned by
cultivar, vintage and climate. Proc Natl Acad Sci 111:E139–
E148
Bolay A (2005) Powdery mildews of Switzerland (Erysiphaceae).
Cryptogr Helv 20:1–176
Booth C (1966) The genus Cylindrocarpon. Mycol Pap 104:1–56
Brasier CM, Sanchez-Hernandez E, Kirk SA (2003) Phytophthora
inundata sp. nov., a part heterothallic pathogen of trees and
shrubs in wet or flooded soils. Mycol Res 107:477–484
Braun U (1998) A monograph of Cercosporella, Ramularia and allied
genera (Phytopathogenic Hyphomycetes), vol 2. IHW-Verlag,
Eching, p 337
Braun U, Crous PW, Dugan F, Groenewald JE, De Hoog GS (2003)
Phylogeny and taxonomy of Cladosporium-like hyphomycetes,
including Davidiella gen. nov., the teleomorph of Cladosporium
s. str. Mycol Prog 2:3–18
Brenckle JF (1918) North Dakota fungi—II. Mycologia 10:199–221
Briceno EX, Latorre BA (2007) Outbreaks of Cladosporium rot
associated with delayed harvest wine grapes in Chile. Plant Dis
91:1060
Briceno EX, Latorre BA (2008) Characterization of Cladosporium rot
in grapevines, a problem of growing importance in Chile. Plant
Dis 92:1635–1642
Bucher VVC, Hyde KD, Pointing SB, Reddy CA (2004) Production
of wood decay enzymes, mass loss and lignin solubilization in
wood by marine ascomycetes and their anamorphs. Fungal
Divers 15:1–14
Burdsall HH Jr (1976) A new species of Laeticorticium (Aphyllophorales, Corticiaceae) from the southern Appalachians.
J Elisha Mitchell Sci Soc 91:243–245
Burdsall HH Jr (1985) A contribution to the taxonomy of the genus
Phanerochaete. Mycol Mem 10:1–165
Burgess TI, Barber PA, Hardy J (2005) Bothryosphaeria spp.
associated with Eucalyptus in Western Australia including
description of Fusicoccum macroclavatum sp. nov. Australas
Plant Pathol 34:557–567
Buritica P (1999) La familia Phakopsoraceae en el neotropico III,
generos: Batistopsora y Phakopsora. Rev Acad Colomb Cienc
23:271–305
Buritica P, Pardo Cardona VM (1996) Flora Uredineana Colombiana.
Rev Acad Colomb Cienc 20:183–236
Cai L, Udayanga D, Manamgoda DS, Maharachchikumbura SSN,
McKenzie EHC, Guo LD, Liu XZ, Bahkali A, Hyde KD (2011)
123
70
The need to carry out re-inventory of plant pathogenic fungi.
Trop Plant Pathol 36:205–213
Campbell WA, Miller JH, Thompson GE (1950) Notes on some
wood-decaying fungi of Georgia. Plant Dis Rep 34:128–134
Candolfi-Arballo O, Valenzuela-Solano C, Gubler WD, HernándezMartı́nez R (2010) Botryosphaeriaceae species associated with
grapevine decline in Mexico. Phytopathol Mediterr 49:105–106
Cannon PF, Hawksworth DL, Sherwood-Pike MA (1985) The British
ascomycotina: An annotated checklist. Commonwealth Mycological Institute, Kew, Surrey
Caporaso JG, Kuczynski J, Stombaugh J, Bittinger K, Bushman FD,
Costello EK, Fierer N, Peña AG, Goodrich JK, Gordon JI,
Huttley GA (2010) QIIME allows analysis of high-throughput
community sequencing data. Nat Methods 7:335–336
Carlucci A, Frisullo S (2009) First report of Diplodia corticola on
grapevine in Italy. J Plant Pathol 91:231–240
Carlucci A, Cibelli F, Lops F, Raimondo ML (2015) Characterization
of Botryosphaeriaceae species as causal agents of trunk disease
on Grapevines. Plant Dis 99:1678–1688
Carlucci A, Lops F, Mostert L, Halleen F, Raimondo ML (2017)
Occurrence fungi causing black foot on young grapevines and
nursery rootstock plants in Italy. Phytopathol Mediterr 56:10–39
Carmaran CC, Novas MV (2003) A review of spegazzini taxa of
Periconia and Sporocybe after over 115 years. Fungal Divers
14:67–76
Carraro L, Maifreni M, Bartolomeoli I, Martino ME, Novelli E, Frigo
F, Marino M, Cardazzo B (2011) Comparison of culturedependent and -independent methods for bacterial community
monitoring during Montasio cheese manufacturing. Res Microbiol 162:231–239
Carter MV (1991) The status of Eutypa lata as a pathogen.
Phytopathol Pap 32:1–59
Cash EK (1952) A record of the fungi named by J.B. Ellis (Part 1).
U.S.D.A. Spec Publ 2:1–165
Cash EK (1953) A record of the fungi named by J.B. Ellis (Part 2).
U.S.D.A. Spec Publ 2:167–345
Cash EK (1954) A record of the fungi named by J.B. Ellis (Part 3).
U.S.D.A. Spec Publ 2:347–518
Casieri L, Hofstetter V, Viret O, Gindro K (2009) Fungal communities living in the wood of different cultivars of young Vitis
vinifera plants. Phytopathol Mediterr 48:73–83
Castellani E, Ciferri R (1937) Prodromus Mycoflorae Africae
Orientalis Italicae. Istituto Agricolo Coloniale Italiano, Firenze
Castillo-Pando M, Somers A, Green CD, Priest M, Sriskathades M
(2001) Fungi associated with dieback of Semillon grapevines in
the Hunter Valley of New South Wales. Australas Plant Pathol
30:59–63
Cavara F (1888) Intorno al disseccamento dei grappoli della vite. Atti
dell’Istituto Botanico della Università e Laboratorio Crittogamico di Pavia 1:293–324
Cavara F (1889) I Funghi Parassiti delle Piante Coltivate ed Utili
Essicati, Delineati e Descriti: 21
Chandra S (1974) Some new leaf-spot diseases from Allahabad
(India). Nova Hedwig 47:35–102
Chardon CE, Toro RA (1930) Mycological explorations of Colombia.
J Dept Agric Porto Rico 14:195–369
Chatasiri S, Ono Y (2008) Phylogeny and taxonomy of the Asian
grapevine leaf rust fungus, Phakopsora euvitis, and its allies
(Uredinales). Mycoscience 49:66–74
Chebil S, Fersi R, Yakoub A, Chenenaoui S, Chattaoui M, Melki I,
Zemni H, Rhouma A, Durante G, Zacchi E, Mliki A (2014) First
report of Botryosphaeria dothidea, Diplodia seriata, and Neofusicoccum luteum associated with canker and dieback of
grapevines in Tunisia. Plant Dis 98:420
Checa J (2004) Dictyosporic Dothideales. Flora Mycol Iber 6:1–162
123
Fungal Diversity (2018) 90:1–84
Chen Q, Jiang JR, Zhang GZ, Cai L, Crous PW (2015) Resolving the
Phoma enigma. Stud Mycol 82:137–217
Chethana KWT, Zhou Y, Zhang W, Liu M, Xing QK, Li XH, Yan JY
(2017) Coniella vitis sp. nov. is the common pathogen of white
rot in Chinese vineyards. Plant Dis 101:2123–2136
Chiarappa L (1959) Wood decay of the grapevine and its relationship
with black measles disease. Phytopathology 49:510–519
Chicau G, Aboim-Inglez M, Cabral S, Cabral JPS (2000) Phaeoacremonium chlamydosporum and Phaeoacremonium angustius
associated with esca and grapevine decline in Vinho Verde
grapevines in northwest Portugal. Phytopathol Mediterr
39:80–86
Cho WD, Shin HD (eds) (2004) List of plant diseases in Korea, 4th
edn. Korean Society of Plant Pathology, Suwon
Chomnunti P, Hongsanan S, Aguirre-Hudson B, Tian Q, Peršoh D,
Dhami MK, Alias AS, Xu J-C, Liu X-Z, Stadler M, Hyde KD
(2014) The sooty moulds. Fungal Divers 66:1–36
Choueiri E, Jreijiri F, Chlela P, Louvet G, Lecomte P (2006)
Occurrence of grapevine decline and first report of black dead
arm associated with Botryosphaeria obtusa in Lebanon. Plant
Dis 90:115
Choueiri E, Jreijiri F, El Amil R, Chlela P, Bugaret Y, Liminana JM,
Mayet V, Lecomte P (2009) First report of black foot disease
associated with Cylindrocarpon sp. in Lebanon. J Plant Pathol
91:231–240
Chupp C (1953) Monograph of the fungus genus Cercospora. Author,
Ithaca
Ciferri R (1929) Micoflora Domingensis. Lista de los hongos hasta la
fecha indicados en Santo Domingo. Publ Estac Estac Agron
Moca Ser B Bot 14:1–260
Ciferri R (1961) Mycoflora Domingensis Integrata. Quaderno
19:1539
Cinelli T, Mondello V, Marchi G, Burruano S, Alves A, Mugnai L
(2016) First report of Diaporthe eres associated with cane blight
of grapevine (Vitis vinifera) in Italy. Plant Dis 100:532
Cloete M, Fischer M, Mostert L, Halleen F (2014) A novel
Fomitiporia species associated with esca on grapevine in South
Africa. Mycol Prog 13:303–311
Cloete M, Fischer M, Mostert L, Halleen F (2015) Hymenochaetales
associated with esca-related wood rots on grapevine with a
special emphasis on the status of esca in South African
vineyards. Phytopathol Mediterr 54:299–312
Cloete M, Fischer M, Du Plessis IL, Mostert L, Halleen F (2016) A
new species of Phellinus sensu stricto associated with esca on
grapevine in South Africa. Mycol Prog 15:25
Comont G, Mayet V, Corio-Costet MF (2016) First report of
Lasiodiplodia viticola, Spencermartinsia viticola and Diplodia
intermedia associated with Vitis vinifera grapevine decline in
French vineyards. Plant Dis 100:2328
Cook RP, Dubé AJ (1989) Host–pathogen index of plant diseases in
South Australia. South Australian Department of Agriculture,
Adelaide
Cooke MC (1878) Ravenel’s American fungi. Grevillea 6:129–146
Cooke WB (1983) The 1979 Oklahoma foray. Mycologia 75:752–755
Correia KC, Camara MPS, Barbosa MAG, Sales R, Agusti-Brisach C,
Gramaje D, Leon M, Garcia-Jimenez J, Abad-Campos P,
Armengol J, Michereff SJ (2013) Fungal trunk pathogens
associated with table grape decline in Northeastern Brazil.
Phytopathol Mediterr 52:380–387
Correia KC, Silva MA, Netto MSB, Vieira WAS, Camara MPS,
Michereff SJ (2016a) First report of grapevine dieback caused by
Neoscytalidium hyalinum in Brazil. Plant Dis 100:213
Correia KC, Silva MA, de Morais Jr MA, Armengol J, Phillips AJL,
Camara MPS, Michereff SJ (2016b) Phylogeny, distribution and
pathogenicity of Lasiodiplodia species associated with dieback
Fungal Diversity (2018) 90:1–84
of table grape in the main Brazilian exporting region. Plant
Pathol 65:92–103
Costa MEA, Camara MS (1952) Species Aliquae Mycologicae
Lusitaniae. Portugaliae Acta Biol Ser A 3:294–307
Coutinho IBL, Freire FCO, Lima CS, Lima JS, Goncalves FJT,
Machado AR, Silva AMS, Cardoso JE (2017) Diversity of genus
Lasiodiplodia associated with perennial tropical fruit plants in
northeastern Brazil. Plant Pathol 66:90–104
Crane JL, Shearer CA (1991) A nomenclator of Leptosphaeria V.
Cesati & G. DeNotaris. Ill Nat Hist Surv Biol Notes 34:1–355
Crous PW, Braun U (2003) Mycosphaerella and its anamorphs: 1.
Names published in Cercospora and Passalora. Centraalbureau
voor Schimmelcultures, Utrecht
Crous PW, Gams W (2000) Phaeomoniella chlamydospora gen. et
comb. nov., a causal organism of Petri grapevine decline and
esca. Phytopathol Mediterr 39:112–118
Crous PW, Braun U, Wingfield MJ, Wood AR, Shin HD, Summerell
BA, Alfenas AC, Cumagun CJR, Groenewald JZ (2009)
Phylogeny and taxonomy of obscure genera of microfungi.
Persoonia 22:139–161
Crous PW, Wingfield MJ, Guarro J, Hernandez-Restrepo M, Sutton
DA, Acharya K, Barber PA, Boekhout T, Dimitrov RA, Duenas
M, Dutta AK, Gene J, Gouliamova DE, Groenewald M,
Lombard L, Morozova OV, Sarkar J, Smith MTh, Stchigel
AM, Wiederhold NP, Alexandrova AV, Antelmi I, Armengol J,
Barnes I, Cano-Lira JF, Castaneda-Ruiz RF, Contu M, PrR
Courtecuisse, da Silveira AL, Decock CA, de Goes A, Edathodu
J, Ercole E (2015) Fungal Planet description sheets: 320–370.
Persoonia 34:167–266
Crous PW, Wingfield MJ, Burgess TI, St J Hardy GE, Barber PA,
Alvarado P, Barnes CW, Buchanan PK, Heykoop M, Moreno G,
Thangavel R, van der Spuy S, Barili A, Barrett S, Cacciola SO,
Cano-Lira JF, Crane C, Decock C, Gilbertoni TB, Guarro J,
Guevara-Suarez M, Hubka V, Kolarik M, Lira CRS, Ordonez
ME, Padamsee M, Ryvarden L, Soares AM, Stchigel AM, Sutton
DA, Vizzini A, Weir BS, Acharya K, Aloi F (2017) Fungal
Planet description sheets: 558–624. Persoonia 38:240–384
Cruywagen EM, Slippers B, Roux J, Wingfield MJ (2017) Phylogenetic species recognition and hybridisation in Lasiodiplodia: a
case study on species from baobabs. Fungal Biol 121:420–436
Cunningham GH (1965) Polyporaceae of New Zealand. Bull N Z
Dept Ind Res 164:1–304
Cunnington J (2003) Pathogenic fungi on introduced plants in
Victoria. A host list and literature guide for their identification.
Department of Primary Industries, Victoria
Cunnington JH, Priest MJ, Powney RA, Cother NJ (2007) Diversity
of Botryosphaeria species on horticultural plants in Victoria and
New South Wales. Australas Plant Pathol 36:157–159
da Silva MA, Correia KC, Barbosa MAG, Camara MPS, Gramaje D,
Michereff SJ (2017) Characterization of Phaeoacremonium
isolates associated with petri disease of table grape in Northeastern Brazil, with description of Phaeoacremonium nordesticola sp. nov. Eur J Plant Pathol 149:695–709
Daamen RA, Langerak CJ, Stol W (1991) Surveys of cereal diseases
and pests in the Netherlands 3. Monographella nivalis and
Fusarium spp. in winter wheat fields and seed lots. Neth J Plant
Pathol 97:105–114
Damm U, Crous PW, Fourie PH (2007) Botryosphaeriaceae as
potential pathogens of Prunus species in South Africa, with
descriptions of Diplodia africana and Lasiodiplodia plurivora
sp. nov. Mycologia 99:664–680
Damm U, Woudenberg JHC, Cannon PF, Crous PW (2009)
Colletotrichum species with curved conidia from herbaceous
hosts. Fungal Divers 39:45–87
71
Damm U, Cannon PF, Woudenberg JHC, Crous PW (2012) The
Colletotrichum acutatum species complex. Stud Mycol
73:37–113
Daranagama DA, Camporesi E, Jeewon R, Liu XZ, Stadler M,
Lumyong S, Hyde KD (2016) Taxonomic rearrangement of
Anthostomella (Xylariaceae) based on a multigene phylogeny
and morphology. Cryptogam Mycol 37:509–538
de Sousa Dias MR, Lucas MT (1972) Fungi Lusitaniae XXIII. Agron.
Lusit 33:173–184
de Sousa Dias MR, Lucas MT, Lopes MC (1987) Fungi Lusitaniae
XXX. Agron Lusit 42:179–188
de Wet J, Slippers B, Preisig O, Wingfield BD, Tsopelas P, Wingfield
MJ (2009) Molecular and morphological characterization of
Dothiorella casuarinae sp. nov. and other Botryosphaeriaceae
with diplodia-like conidia. Mycologia 101:503–511
Deighton FC (1976) Studies on Cercospora and allied genera. VI.
Pseudocercospora Speg., Pantospora Cif. and Cercoseptoria
Petr. Mycol Pap 140:1–168
Deighton J (2016) Fungi in ecosystem processes, vol 31. CRC Press,
Boca Raton
Denaree JB, Runner GA (1942) Control of grape diseases and insects
in Eastern United States. Diseases principally of Amaerican
bunch grapes. US Dept Agr Farm Bull 1893:1–28
Dennis RWG (1964) Remarks on the genus Hymenoscyphus S.F.
Gray, with observations on sundry species referred by Saccardo
and others to the genera Helotium Pezizella or Phialea.
Persoonia 3:29–80
Dennis RWG (1970) Kew Bulletin Additional Series III. Fungus flora
of Venezuela and adjacent countries. Verlag von J Cramer,
Weinheim
Diaz GA, Latorre BA (2014) Infection caused by Phaeomoniella
chlamydospora associated with esca-like symptoms in grapevine
in Chile. Plant Dis 98:351–360
Diaz GA, Prehn D, Latorre BA (2011) First report of Cryptovalsa
ampelina and Eutypella leprosa associated with grapevine trunk
diseases in Chile. Plant Dis 95:490
Diaz GA, Elfar K, Latorre BA (2012) First report of Seimatosporium
botan associated with trunk disease of grapevine (Vitis vinifera)
in Chile. Plant Dis 96:1696
Diaz G, Auger J, Besoain X, Bordeu E, Latorre BA (2013) Prevalence
and pathogenicity of fungi associated with grapevine trunk
diseases in Chilean vineyards. Cien Inv Agr 40:327–339
Dingley JM, Fullerton RA, McKenzie EHC (1981) Survey of
agricultural pests and diseases. Technical Report, vol 2. Records
of fungi, bacteria, algae, and angiosperms pathogenic on Plants
in Cook Islands, Fiji, Kiribati, Niue, Tonga, Tuvalu, and Western
Samoa. F.A.O., Rome
Dissanayake AJ, Zhang W, Mei L, Chukeatirote E, Yan JY, Li XH,
Hyde KD (2015) Lasiodiplodia pseudotheobromae causes
pedicel and peduncle discolouration of grapes in China.
Australas Plant Pathol 10:21
Dissanayake AJ, Purahong W, Wubet T, Hyde KD, Wei Z, Xu HY,
Zhang GJ, Yuan FC, Liu M, Xing Q, Li XH, Yan JY (2018)
Direct comparison of culture dependent and cultire independent
molecular approaches reveal the diversity of fungal endophytic
communities in stems of grapevine (Vitis vinifera). Fungal
Divers (Under review)
Dohadwala MM, Vita JA (2009) Grapes and Cardiovascular Disease.
J Nutr 139:1788S–1793S
Doidge EM (1950) The South African fungi and lichens to the end of
(1945). Bothalia 5:1–1094
Doilom MW, Shuttleworth LA, Roux J, Chukeatirote E, Hyde KD
(2015) Botryosphaeriaceae associated with Tectona grandis
(teak) in northern Thailand. Phytotaxa 233:1–26
123
72
Du Z, Fan X-L, Hyde KD, Yang Q, Liang Y-M, Tian C-M (2016)
Phylogeny and morphology reveal two new species of Diaporthe
form Betula spp. in China. Phytotaxa 269:090–102
Duarte S, Pascoal C, Cássio F, Bärlocher F (2006) Aquatic
hyphomycete diversity and identity affect leaf litter decomposition in microcosms. Oecologia 147:658–666
Dudka IO, Heluta VP, Tykhonenko YY, Andrianova TV, Hayova VP,
Prydiuk MP, Dzhagan VV, Isikov VP (2004) Fungi of the
Crimean Peninsula. M.G. Kholodny Institute of Botany, National
Academy of Sciences of Ukraine, Kiev
Dugan FM, Schubert K, Braun U (2004) Check-list of Cladosporium
names. Schlechtendalia 11:1–103
Dupont J, Laloui W, Roquebert MF (1998) Partial ribosomal DNA
sequences show an important divergence between Phaeoacremonium species isolated from Vitis vinifera. Mycol Res
102:631–637
Dupont J, Laloui W, Magnin S, Larignon P, Roquebert M-F (2000)
Phaeoacremonium viticola, a new species associated with Esca
disease of grapevine in France. Mycologia 92:499–504
Dupont J, Magnin S, Cesari C, Gatica M (2002) ITS and b-tubulin
markers help delineate Phaeoacremonium species, and the
occurrence of P. parasiticum in grapevine disease in Argentina.
Mycol Res 106:1143–1150
Ebbels DL, Allen DJ (1979) A supplementary and annotated list of
plant diseases, pathogens and associated fungi in Tanzania.
Phytopathol Pap 22:1–89
Edgar RC (2004) Muscle: a multiple sequence alignment method with
reduced time and space complexity. BMC Bioinformatics 5:113
Edgar RC (2013) UPARSE: highly accurate OTU sequences from
microbial amplicon reads. Nat Methods 10:996–998
Edgar RC, Haas BJ, Clemente JC, Quince C, Knight R (2011)
UCHIME improves sensitivity and speed of chimera detection.
Bioinformatics 27:2194–2200
El-Buni AM, Rattan SS (1981) Check list of Libyan Fungi. Al Faateh
University, Fac Sci, Dept. Bot, Tripoli
Elenkin AA (1909) Title unknown. Bolezni Rast 4:68
Ellis JB, Everhart BM (1904) New species of fungi from various
localities. J Mycol 10:167–170
Epstein L (2008) Botryosphaeria-related dieback and control investigated in noncoastal California grapevines. Calif Agric
62:161–166
Erwin DC, Ribeiro OK (1996) Phytophthora diseases worldwide. APS
Press, St. Paul
Esfandiari E, Petrak F (1950) Pilze aus Iran. Sydowia 4:11–38
Eskalen A, Rooney-Latham S, Gubler WD (2005) First report of
perithecia of Phaeoacremonium viticola on grapevine (Vitis
vinifera) and ash tree (Fraxinus latifolia) in California. Plant Dis
89:686–686
Essakhi S, Mugnai L, Crous PW, Groenewald JZ, Surico G (2008)
Molecular and phenotypic characterisation of novel Phaeoacremonium species isolated from esca diseased grapevines. Persoonia 21:119–134
Fadrosh DW, Ma B, Gajer P, Sengamalay N, Ott S, Brotman RM,
Ravel J (2014) An improved dual-indexing approach for
multiplexed 16S rRNA gene sequencing on the Illumina MiSeq
platform. Microbiome 2:6
Faedda R, Agosteo GE, Schena L, Mosca S, Frisullo S, di San
Magnano, Lio G, Cacciola SO (2011) Colletotrichum clavatum
sp. nov. identified as the causal agent of olive anthracnose in
Italy. Phytopathol Mediterr 50:283–302
Farr ML (1973) An annotated list of Spegazzini’s fungus taxa, Vol. 1.
Biblioth Mycol 35:1–823
Farr DF, Castlebury LA, Rossman AY, Erincik O (2001) Greeneria
uvicola, cause of bitter rot of grapes, belongs in the Diaporthales.
Sydowia 53:185–199
123
Fungal Diversity (2018) 90:1–84
Farr DF, Elliott M, Rossman AY, Edmonds RL (2005) Fusicoccum
arbuti sp. nov. causing cankers on Pacific madrone in western
North America with notes on Fusicoccum dimidiatum, the
correct name for Scytalidium dimidiatum and Nattrassia
mangiferae. Mycologia 97:730–741
Fautrey F, Lambotte JBE (1896) Espèces nouvelles ou rares de la
Côte d’Or. Revue Mycologique Toulouse. 18:68–71
Ferrada EE, Diaz GA, Zoffoli JP, Latorre BA (2014) First report of
blossom blight caused by Sclerotinia sclerotiorum on Japanese
plum, nectarine, and sweet cherry orchards in Chile. Plant Dis
98:695
Fischer M, Edwards J, Cunnington JH, Pascoe IG (2005) Basidiomycetous pathogens on grapevine: a new species from
Australia—Fomitiporia australiensis. Mycotaxon 92:85–96
Fischer M, Schneider P, Kraus C, Molnar M, Dubois C, D’Aguiar D,
Haag N (2016) Grapevine trunk disease in German viticulture:
occurence of lesser known fungi and first report of Phaeoacremonium viticola and P. fraxinopennsylvanicum. Vitis
55:145–156
Fitt BD, Brun H, Barbetti MJ, Rimmer SR (2006) World-wide
importance of phoma stem canker (Leptosphaeria maculans and
L. biglobosa) on oilseed rape (Brassica napus). In: Fitt BDL,
Evans N, Howlett BJ, Cooke BM (eds) Sustainable strategies for
managing Brassica napus (oilseed rape) resistance to Leptosphaeria maculans (phoma stem canker). Springer, Dordrecht,
pp 3–15
Foister CE (1961) The economic plant diseases of Scotland. Techn
Bull Dept Agric Fish Scotland 1:1–210
Forster H, Coffey MD (1993) Molecular taxonomy of Phytophthora
megasperma based on mitochondrial and nuclear DNA polymorphisms. Mycol Res 97:1101–1112
Fotouhifar K-B, Hedjaroude G-A, Leuchtmann A (2010) ITS rDNA
phylogeny of Iranian strains of Cytospora and associated
teleomorphs. Mycologia 102:1369–1382
Fourie PH, Halleen F (2002) Investigation on the occurence of
Phaeomoniella chlamydospora in canes of rootstock mother
vines. Australas Plant Pathol 31:425–426
Fournier E, Gladieux P, Giraud T (2013) The ‘Dr Jekyll and Mr Hyde
fungus’: noble rot versus gray mold symptoms of Botrytis
cinerea on grapes. Evol Applic 6:960–969
French AM (1987) California plant disease host index. Part 1: fruit
and nuts. California Department of Food Agriculture,
Sacramento
French AM (1989) California plant disease host index. California
Department of Food Agriculture, Sacramento
Gadgil PD (2005) Fungi on trees and shrubs in New Zealand. In:
Fungi of New Zealand, vol 4. Fungal Diversity Press, Hong
Kong
Gao Z-M, Li Y-M, Li X-L, Zhang Z-H, Yiny J-F (2009) Comparison
of the biological characteristics of Botrytis cinerea isolates from
different hosts. Mycosystema 28:370–377
Gaponenko NI (1965) Survey of the fungi of Bukhara. Akad Sa
Uzbekh
Garcı́a B, López L, Velázquez M, Pérez-Moreno J (1998) Mycorrhizal and saprotrophic macrofungi in declining sacred-fir stands.
Micol Neotrop Apl 11:9–21
Garcia-Benavides P, Martin Zamorano P, Ocete Perez CA, Maistrello
L, Ocete Rubio R (2013) Biodiversity of pathogenic wood fungi
isolated from Xylotrechus arvicola (Olivier) galleries in vine
shoots. J Int Sci Vigne Vin 47:73–81
Garcia-Blazquez G, Constantinescu O, Telleria MT, Martin MP
(2006) Preliminary checklist of Albuginales and Peronosporales
(Chromista) reported from the Iberian Peninsula and Balearic
Islands. Mycotaxon 98:185–188
Garnica S, Riess K, Schön ME, Oberwinkler F, Setaro SD (2016)
Divergence times and phylogenetic patterns of Sebacinales, a
Fungal Diversity (2018) 90:1–84
highly diverse and widespread fungal lineage. PLoS ONE
11:e0149531
Gatica M, Cesari C, Magnin S, Dupont J (2001) Phaeoacremonium
species and Phaeomoniella chlamydospora in vines showing
‘‘hoja de malvon’’ and young vine decline symptoms in
Argentina. Phytopathol Mediterr 40:S317–S324
Ge Q, Chen Y, Xu T (2009) Flora Fungorum Sinicorum. Pestalotiopsis, vol 38. Science Press, Beijing, p 235
Georghiou GP, Papadopoulos C (1957) A second list of Cyprus fungi.
Government of Cyprus, Department of Agriculture, Nicosia
Gerlach W, Ershad D (1970) Beitrag zur Kenntnis der Fusarium und
Cylindrocarpon-Arten in Iran. Nova Hedwig 20:725–784
Giatgong P (1980) Host index of plant diseases in Thailand, 2nd edn.
Mycology Branch, Plant Pathology and Microbiology Division,
Department of Agriculture and Cooperatives, Bangkok
Gilbertson RL, Martin KJ, Lindsey JP (1974) Annotated check list
and host index for Arizona wood-rotting fungi. Univ Arizona
Agric Exp Sta Techn Bull 209:1–48
Gilman JC (1932) First supplementary list of parasitic fungi from
Iowa. Iowa State Coll J Sci 6:357–365
Gilman JC, Archer WA (1929) The Fungi of Iowa Parasitic on Plants.
Iowa State Coll J Sci 3:299–507
Gimenez-Jaime A, Aroca A, Raposo R, Garcia-Jimenez J, Armengol J
(2006) Occurrence of fungal pathogens associated with grapevine nurseries and the decline of young vines in Spain.
J Phytopathol 154:598–602
Gomes RR, Glienke C, Videira SIR, Lombard L, Groenewald JZ,
Crous PW (2013) Diaporthe: a genus of endophytic, saprobic
and plant pathogenic fungi. Persoonia 31:1–41
Gonzalez CD, Chaverri P (2017) Corinectria, a new genus to
accommodate Neonectria fuckeliana and C. constricta sp. nov.
from Pinus radiata in Chile. Mycol Prog 16(11–12):1015–1027
Gonzalez Fragoso R (1916) Bosquejo de una Florula Hispalense de
Micromicetos. Trab Mus Nac Ci Nat Ser Bot 10:1–221
Gonzalez Fragoso R (1917) Fungi novi vel minus cognitarum horti
botanici matritense. Trab Mus Nac Ci Nat Ser Bot 12:1–99
Gonzalez Fragoso R (1921) Algunos Demaciaceos de la Flora
espanola. Bol Real Soc Esp Hist Nat 21:93–99
Gonzalez V, Tello ML (2011) The endophytic mycota associated with
Vitis vinifera in central Spain. Fungal Diver 47:29–42
Goos RD (2010) The Mycota of Rhode Island: a checklist of the fungi
recorded in Rhode Island (including lichens and myxomycetes).
R I Nat Hist Surv 4:222
Gorter GJMA (1977) Index of plant pathogens and the diseases they
cause in cultivated plants in South Africa. Republic South Africa
Dept Agric Techn Serv. Pl Protect Res Inst Sci Bull 392:1–177
Graham AB, Johnston PR, Weir BS (2009) Three new Phaeoacremonium species on grapevines in New Zealand. Australas Plant
Pathol 38:505–513
Gramaje D, Alaniz S, Perez Sierra A, Abad-Campos P, GarciaJimenez J, Armengol J (2008) First report of Phaeoacremonium
scolyti causing petri disease of grapevine in spain. Plant Dis
92:836
Gramaje D, Armengol J, Mohammadi H, Banihashemi Z, Mostert L
(2009) Novel Phaeoacremonium species associated with petri
disease and esca of grapevine in Iran and Spain. Mycologia
101:920–929
Gramaje D, Aguilar MI, Armengol J (2011) First report of
Phaeoacremonium krajdenii causing petri disease of grapevine
in Spain. Plant Dis 95:615
Grand LF (ed) (1985) North Carolina Plant Disease Index. North
Carolina Agric Res Serv Techn Bull 240:1–157
Grasso S (1984) Infezioni di Fusarium oxysporum e di Cylindrocarpon destructans associate a una moria di giovani piante di vite in
Sicilia. Inf Fitopatol 1:59–63
73
Greene HC (1955) Notes on Wisconsin parasitic fungi. XXI. Trans.
Wisconsin Acad Sci 44:29–43
Greene HC (1956) Notes on Wisconsin parasitic fungi. XXII. Trans.
Wisconsin Acad Sci 45:177–191
Greene HC (1963) Notes on Wisconsin parasitic fungi. XXIX. Trans
Wisconsin Acad Sci 52:229–253
Greene HC (1966) Notes on Wisconsin parasitic fungi. XXXII. Trans
Wisconsin Acad Sci 55:147–166
Greuter W, Poelt J, Raimondo FM (1991) A checklist of Sicillian
fungi. Bocconea 2:222
Guba EF (1961) Monograph of Monochaetia and Pestalotia. Harvard
University Press, Cambridge
Guerber JC, Liu B, Correll JC, Johnston PR (2003) Characterization
of diversity in Colletotrichum acutatum sensu lato by sequence
analysis of two gene introns, mtDNA and intron RFLPs, and
mating compatibility. Mycologia 95:872–895
Guo Y-L, Liu X-J (eds) (2003) Flora Fungorum Sinicorum. Mycovellosiella, Passalora, Phaeoramularia, vol. 20 Science Press,
Beijing
Guo LD, Huang GR, Wang Y, He WH, Zheng WH, Hyde KD (2003)
Molecular identification of white morphotype strains of endophytic fungi from Pinus tabulaeformis. Mycol Res 107:680–688
Haas BJ, Gevers D, Earl AM, Feldgarden M, Ward DV, Giannoukos
G, Ciulla D, Tabbaa D, Highlander SK, Sodergren E, Methé B
(2011) Chimeric 16S rRNA sequence formation and detection in
Sanger and 454-pyrosequenced PCR amplicons. Genome Res
21:494–504
Halleen F, Crous PW, Petrini O (2003) Fungi associated with healthy
grapevine cuttings in nurseries, with special reference to
pathogens involved in the decline of young vines. Australas
Plant Pathol 32:47–52
Hammer Ø, Harper DAT, Ryan PD (2001) PAST: paleontological
statistics software package for education and data analysis.
Palaeontol Electron 4:1–9
Hanlin RT (1963) A revision of the Ascomycetes of Georgia. Georgia
Agric Exp Sta Mimeo Ser ns 175:1–65
Hanlin RT (1966) Host index to the Basidiomycetes of Georgia.
Georgia Agric Exp Sta Mimeo Ser ns 260:1–30
Hansford CG (1947) New or interesting tropical fungi—I. Proc Linn
Soc London 158:28–50
Hanson CA, Fuhrman JA, Horner-Devine MC, Martiny JBH (2012)
Beyond biogeographic patterns:processes shaping the microbial
landscape. Nat RevMicrobiol 10:497–506
Harvey JM (1955) A method of forecasting decay in California
storage grapes. Phytopathology 45:229–232
Henricot B, Pérez Sierra A, Prior C (2000) A new blight disease on
Buxus in the UK caused by the fungus Cylindrocladium. Plant
Pathol 49:805–805
Hernandez JC (2004) Bases Corologicas de Flora Micologica Iberica.
Adiciones y numeros 2179–2238. Cuad Trab Fl Micol Iber
20:1–94
Hewitt WB (1951) Grape dead-arm control. Plant Dis Rep
35:142–143
Hewitt WB (2015) Miscellaneous berry rots and raisin molds. In:
Gubler WD, Uyemoto JK (eds) Compendium of grape diseases,
disorders and pests (Wilcox WF. American phytopathological
society, USA, pp 22–24
Hirayama K, Tanaka K (2011) Taxonomic revision of Lophiostoma
and Lophiotrema based on reevaluation of morphological
characters and molecular analyses. Mycoscience 52:401–412
Hirooka Y, Rossman AY, Zhuang W-Y, Salgado-Salazar C, Chaverri
P (2013) Species delimitation for Neonectria coccinea group
including the causal agents of beech bark disease in Asia,
Europe, and North America. Mycosystema 32:485–517
123
74
Hock J, Dittrich U, Renfro BL, Kranz J (1992) Sequential development of pathogens in the maize tarspot disease complex.
Mycopathologia 117:157–161
Hofstetter V, Buyck B, Croll D, Viret O, Couloux A, Gindro K (2012)
What if esca disease of grapevine were not a fungal disease?
Fungal Divers 54:51–67
Holevas CD, Chitzanidis A, Pappas AC, Tzamos EC, Elena K,
Psallidas PG, Alivizatos AS, Panagopoulos CG, Kyriakopoulou
PE, Bem FP, Lazscaris DN (2000) Disease agents of cultivated
plants observed in Greece from 1981 to 1990. Benaki Phytopathol Inst Kiphissia Athens 19:1–96
Hoppe B, Purahong W, Wubet T, Kahl T, Bauhus J, Arnstadt T,
Hofrichter M, Buscot F, Krüger D (2016) Linking molecular
deadwood-inhabiting fungal diversity and community dynamics
to ecosystem functions and processes in Central European
forests. Fungal Divers 77:367–379
Hrustic J, Delibasic G, Stankovic I, Grahovac M, Krstic B, Bulajic A,
Tanovic B (2015) Monilinia spp. causing brown rot of stone fruit
in Serbia. Plant Dis 99:709–717
Hsieh W-H, Goh T-K (1990) Cercospora and similar fungi from
Taiwan. Maw Chang Book, Taipei
Huang F, Udayanga D, Wang X, Hou X, Mei X, Fu Y, Hyde KD, Li
H (2015) Endophytic Diaporthe associated with Citrus: a
phylogenetic reassessment with seven new species from China.
Fungal Biol 119:331–347
Hugenholtz P, Goebel BM, Pace NR (1998) Impact of cultureindependent studies on the 23 emerging phylogenetic view of
bacterial diversity. J Bacteriol 180:4765–4774
Hyde KD, Bussaban B, Paulus B, Crous PW, Lee S, Mckenzie EH,
Photita W, Lumyong S (2007) Diversity of saprobic microfungi.
Biodivers Conserv 16:7–35
Hyde Kevin D, Abd-Elsalam Kamel, Cai Lei (2010) Morphology: still
essential in a molecular world. Mycotaxon 114:439–451
Hyde KD, Nilsson RH, Alias SA, Ariyawansa HA, Blair JE, Cai L, de
Cock AWAM, Dissanayake AJ, Glockling SL, Goonasekara ID,
Gorczak M, Hahn M, Jayawardena RS, van Kan JAL, Laurence
MH, Lévesque CA, Li XH, Liu JK, Maharachchikumbura SSN,
Manamgoda DS, Martin FN, McKenzie EHC, McTaggart AR,
Mortimer PE, Nair PVR, Pawłowska J, Rintoul TL, Shivas RG,
Spies CFJ, Summerell BA, Taylor PWJ, Terhem RB, Udayanga
D, Vaghefi N, Walther G, Wilk M, Wrzosek M, Xu JC, Yan JY,
Zhou N (2014) One stop shop: backbones trees for important
phytopathogenic genera: I. Fungal Divers 67:21–125
Hyde KD, Hongsanan S, Jeewon R, Bhat DJ, McKenzie EHC, Jones
EBG, Phookamsak R, Ariyawansa HA, Boonmee S, Zhao Q,
Abdel-Aziz FA, Abdel-Wahab MA, Banmai S, Chomnunti P,
Cui BK, Daranagama DA, Das K, Dayarathne MC, de Silva NI,
Dissanayake AJ, Doilom M, Ekanayaka AH, Gibertoni TB,
Góes-Neto A, Huang SK, Jayasiri SC, Jayawardena RS, Konta S,
Lee HB, Li WJ, Lin CG, Liu JK, Lu YZ, Luo ZL, Manawasinghe
IS, Manimohan P, Mapook A, Niskanen T, Norphanphoun C,
Papizadeh M, Perera RH, Phukhamsakda C, Richter C, de
Santiago ALCMA, Drechsler-Santos ER, Senanayake IC,
Tanaka K, Tennakoon TMDS, Thambugala KM, Tian Q,
Tibpromma S, Thongbai B, Vizzini A, Wanasinghe DN,
Wijayawardene NN, Wu HX, Yang J, Zeng XY, Zhang H,
Zhang JF, Bulgakov TS, Camporesi E, Bahkali AH, Amoozegar
AM, Araujo-Neta LS, Ammirati JF, Baghela A, Bhatt RP,
Bojantchev S, Buyck B, da Silva GA, de Lima CLF, de Oliveira
RJV, de Souza CAF, Dai YC, Dima B, Duong TT, Ercole E,
Mafalda-Freire F, Ghosh A, Hashimoto A, Kamolhan S, Kang
JC, Karunarathna SC, Kirk PM, Kytövuori I, Lantieri A,
Liimatainen K, Liu ZY, Liu XZ, Lücking R, Medardi G,
Mortimer PE, Nguyen TTT, Promputtha I, Raj KNA, Reck MA,
Lumyong S, Shahzadeh-Fazeli SA, Stadler M, Soudi MR, Su
HY, Takahashi T, Tangthirasunun N, Uniyal P, Wang Y, Wen
123
Fungal Diversity (2018) 90:1–84
TC, Xu JC, Zhang ZK, Zhao YC, Zhou JZ, Zhu L (2016) Fungal
diversity notes 367–490: taxonomic and phylogenetic contributions to fungal taxa. Fungal Divers 80:1–270
Hyde KD, Norphanphoun C, Abreu VP, Bazzicalupo A, Chethana
KT, Clericuzio M, Dayarathne MC, Dissanayake AJ, Ekanayaka
AH, He MQ, Hongsanan S, Huang SK, Jayasiri SC, Jayawardena
RS, Karunarathna A, Konta S, Kušan I, Lee H, Li J, Lin CG, Liu
NG, Lu YZ, Luo ZL, Manawasinghe IS, Mapook A, Perera RH,
Phookamsak R, Phukhamsakda C, Siedlecki I, Soares AM,
Tennakoon D, Tian Q, Tibpromma S, Wanasinghe DN, Xiao YP,
Yang J, Zeng XY, Abdel-Aziz FA, Li WJ, Senanayake IC, Shang
QJ, Daranagama DA, de Silva NI, Thambugala KM, AbdelWahab MA, Bahkali AH, Berbee ML, Boonmee S, Bhat DJ,
Bulgakov TS, Buyck B, Camporesi E, Castañeda-Ruiz RF,
Chomnunti P, Doilom M, Dovana F, Gibertoni TB, Jadan M,
Jeewon R, Jones EBG, Kang JC, Karunarathna SC, Lim YW, Liu
JK, Liu ZY, Plautz HL Jr, Lumyong S, Maharachchikumbura
SSN, Matočec N, McKenzie EHC, MeŠić A, Miller D,
Pawlowska J, Pereira OL, Promputtha I, Romero AI, Ryvarden
L, Su HY, Suetrong S, Tkalčec Z, Vizzini A, Wen TC,
Wisitrassameewong K, Wrzosek M, Xu JC, Zhao Q, Zhao RL,
Mortimer P (2017) Fungal diversity notes 603–708: taxonomic
and phylogenetic notes on genera and species. Fungal Divers
87:1–235
Index Fungorum (2018) http://www.indexfungorum.org/names/
names.asp
Jackson HS (1931) The rusts of South America based on the Holway
collections—V. Mycologia 23:463–503
Jarvis WR, Traquair JA (1984) Bunch rot of grapes caused by
Aspergillus aculeatus. Plant Dis 68:718–719
Javed S, Javaid A, Anwar W, Majeed RA, Akhtar R, Naqvi SF (2017)
First Report of Botrytis Bunch Rot of Grapes Caused by Botrytis
cinerea in Pakistan. Plant Dis 101:1036
Jayawardena RS, Zhang W, Liu M, Maharachchikumbura SSN, Zhou
Y, Huang J-B, Nilthong S, Wang Z-Y, Li XH, Yan JY, Hyde KD
(2015) Identification and characterization of Pestalotiopsis-like
fungi related to grapevine diseases in China. Fungal Biol
119:348–361
Jayawardena RS, Liu M, Maharachchikumbura SS, Zhang W, Xing
Q, Hyde KD, Nilthong S, Li X, Yan J (2016a) Neopestalotiopsis
vitis sp. nov. causing grapevine leaf spot in China. Phytotaxa
258:63–74
Jayawardena RS, Hyde KD, Damm U, Cai L, Liu M, Li XH, Zhang
W, Zhao WS, Yan JY (2016b) Notes on currently accepted
species of Colletotrichum. Mycosphere 7:1192–1260
Jayawardena RS, Hyde KD, Chethana KWT, Daranagama DA,
Dissanayake AJ, Goonasekara ID, Manawasinghe IS, Mapook A,
Jayasiri SC, Karunarathne A, Li C-G, Phukhamsakda C,
Senanayake IC, Wanasinghe DN, Camporesi E, Bulgakov TS,
Li XH, Liu M, Zhang W, Yan JY (2018) Mycosphere Notes
102–168: saprotrophic fungi on Vitis in China, Italy, Russia and
Thailand. Mycosphere 9:1–114
Jeewon R, Hyde KD (2016) Establishing species boundaries and new
taxa among fungi: recommendations to resolve taxonomic
ambiguities. Mycosphere 7:1669–1677
Jenkins AE, Bitancourt AA (1940–1963) Myrangiales Selecti Exsiccati. Nos. 1–550. Exsiccati set
Jones DR, Baker RH (2007) Introductions of non-native plant
pathogens into Great Britain, (1970–2004). Plant Pathol
56:891–910
Ju Y-M, Rogers JD (1995) Pareutypella gen. nov. for two longostiolate pyrenomycetes from Taiwan. Mycologia 87:891–895
Ju Y-M, Rogers JD (1999) The Xylariaceae of Taiwan (excluding
Anthostomella). Mycotaxon 73:343–440
Fungal Diversity (2018) 90:1–84
Kakalikova L, Jankura E, Srobarova A (2009) First report of
Alternaria bunch rot of grapevines in Slovakia. Australas Plant
Pathol 4:68–69
Kamal (2010) Cercosporoid fungi of India. Bishen Singh Mahendra
Pal Singh, Dehra Dun, p 351
Kanagawa T (2003) Bias and artifacts in multitemplate polymerase
chain reaction (PCR). J Biosci Bioengin 96:317–323
Kanematsu S, Minaka N, Kobayashi T, Kudo A, Ohtsu Y (2000)
Molecular phylogenetic analysis of Ribosomal DNA internal
transcribed spacer regions and comparison of fertility in
Phomopsis isolates from fruit trees. J Gen Plant Pathol
66:191–201
Kantschaveli LA (1928) New species of fungi from Georgia. Bolezni
Rastenij 17:81–94
Karimi MR, Mahmoodi B, Kazemiyan M (2001) First report of esca
of grapevine in Iran. Phytopathol Mediterr 40:S481
Kepley JB, Reeves FB, Jacobi WR, Adams GC (2015) Species
associated with Cytospora canker on Populus tremuloides.
Mycotaxon 130:783–805
Kern FD, Thurston HW Jr, Whetzel HH (1934) Uredinales. Monogr
Univ Puerto Rico B 2:262–303
Khan S, Kamal M (1974) Additions to the parasitic fungi of West
Pakistan—III. Mycopathol Mycol Appl 52:29–43
Kim J-D, Shin HD (1998) Taxonomic studies on Cercospora and
allied genera in Korea (I). Korean J Mycol 26:327–341
Kim WK, Sang HK, Woo SK, Park MS, Paul NC, Yu SH (2007) Six
species of Penicillium associated with blue mold of grape.
Mycobiology 35:180–185
Ko TWK, Stephenson SL, Bahkali AH, Hyde KD (2011) From
morphology to molecular biology: can we use sequence data to
identify fungal endophytes? Fungal Divers 50:113
Kobayashi T (2007) Index of fungi inhabiting woody plants in Japan.
Host, distribution and literature. Zenkoku-Noson-Kyoiku Kyokai
Publishing, Tokyo
Koike ST, Bettiga LJ, Nguyen TT, Gubler WD (2016) First report of
Cylindrocladiella lageniformis and C. peruviana as grapevine
pathogens in California. Plant Dis 100:1783–1784
Kõljalg U, Nilsson RH, Abarenkov K, Tedersoo L, Taylor AF,
Bahram M, Bates ST, Bruns TD, Bengtsson-Palme J, Callaghan
TM, Douglas B (2013) Towards a unified paradigm for
sequence-based identification of fungi. Mol Ecol 22:5271–5277
Konstantinia-Sulidu A (1939) Parasitische Pilze Mazedoniens. Hedwig 78:284–298
Korf RP, Pearson RC, Zhuang WY, Dubos B (1986) Pseudopezicula
(Helotiales, Peziculoideae), a new discomycete genus for
pathogens causing an angular leaf scorch of grapes (‘‘Rotbrenner’’). Mycotaxon 26:457–471
Koshkelova EN, Frolov IP (1973) Microflora of Kopet-Dag lowland
and Central Karakum (micromycetes). Ylym, Ashkhabad
Kotlaba F (1997) Some uncommon or rare polypores (Polyporales
s.l.) collected on uncommon hosts. Czech Mycol 50:133–142
Kozich JJ, Westcott SL, Baxter NT, Highlander SK (2013) Schloss
PD: development of a dual-index sequencing strategy and
curation pipeline for analyzing amplicon sequence data on the
MiSeq Illumina sequencing platform. Appl Environ Microbiol
79:5112–5120
Kubatova A, Kolarik M, Pazoutova S (2004) Phaeoacremonium
rubrigenum-Hyphomycete associated with bark beetles found in
Czechia. Folia Microbiol 49:99–104
Kubartova A, Ottosson E, Dahlberg A, Stenlid J (2012) Patterns of
fungal communities among and within decaying logs, revealed
by 454sequencing. Mol Ecol 21:4514–4532
Kummuang N, Smith BJ, Diehl SV, Graves CH Jr (1996) Muscadine
grape berry rot diseases in Mississippi: disease identification and
incidence. Plant Dis 80:238–243
75
Kunin V, Engelbrektson A, Ochman H, Hugenholtz P (2010)
Wrinkles in the rare biosphere: pyrosequencing errors can lead
to artificial inflation of diversity estimates. Environ Microbiol
12:118–123
Kuntze O (1898) Revisio generum plantarum: vascularium omnium
atque cellularium multarum secundum leges nomeclaturae
internationales cum enumeratione plantarum exoticarum in
itinere mundi collectarum. A. Felix 3:1–576
Kuo K-C, Leu L-S (1998) Phomopsis vitimegaspora: a new
pathogenic Phomopsis from vines. Mycotaxon 66:497–499
Lane C, Kirk P (2012) Introduction to fungal plant pathogens. CAB
International, Cambridge, pp 1–6
Langrell SRH, Morel O, Robin C (2011) Touchdown nested multiplex
PCR detection of Phytophthora cinnamomi and P. cambivora
from French and English chestnut grove soils. Fungal Biol
115:672–682
Lardner R, Stummer BE, Sosnowski MR, Scott ES (2005) Molecular
identification and detection of Eutypa lata in grapevine. Mycol
Res 109:799–808
Larignon P, Dubos B (1997) Fungi associated with esca disease in
grapevine. Eur J Plant Pathol 103:147–157
Larignon P, Dubos B (2001) The villainy of black dead arm. Wines
Vines 82:86–89
Larsen MJ, Nakasone KK (1984) Additional new taxa of Laeticorticium (Aphyllophorales, Corticiaceae). Mycologia 76:528–532
Larter LNH, Martyn EB (1943) A preliminary list of plant diseases in
Jamaica. Mycol Pap 8:1–16
Latorre BA, Guerrero MJ (2001) First report of shoot blight of
grapevine caused by Sclerotinia sclerotiorum in Chile. Plant Dis
85:1122
Lawrence DP, Travadon R, Baumgartner K (2015) Diversity of
Diaporthe species associated with wood cankers of fruit and nut
crops in northern California. Mycologia 107:926–940
Lawrence DP, Travadon R, Pouzoulet J, Rolshausen PE, Wilcox WF,
Baumgartner K (2017a) Characterization of Cytospora isolates
from wood cankers of declining grapevine in North America,
with the descriptions of two new Cytospora species. Plant Pathol
66:713–725
Lawrence DP, Peduto Hand F, Gubler WD, Trouillas FP (2017b)
Botryosphaeriaceae species associated with dieback and canker
disease of bay laurel in northern California with the description
of Dothiorella californica sp. nov. Fungal Biol 121:347–360
Lee Y-H, Cho W-D, Kim WK, Jin K-S, Lee E-J (1991) Report on
host-unrecorded diseases identified from economical crops in
Korea. Res Rep Rural Developm Admin 33:15–19
Li W, Liu J, Bhat DJ, Camporesi E, Xu J, Hyde KD (2014)
Introducing the novel species, Dothiorella symphoricarposicola,
snowberry in Italy. Cryptog Mycol 35:257–270
Li GJ, Hyde KD, Zhao RN, Hongsanan S, Abdel-Aziz FA,
AbdelWahab MA, Alvarado P, Alves-Silva G, Ammirati JF,
Ariyawansa HA, Baghela A, Bahkali AH, Beug M, Bhat DJ,
Bojantchev D, Boonpratuang T, Bulgakov TS, Camporesi E,
Boro MC, Ceska O, Chakraborty D, Chen JJ, Chethana KWT,
Chomnunti P, Consiglio G, Cui BK, Dai DQ, Dai YC,
Daranagama DA, Das K, Dayarathne MC, Crop ED, De Oliveira
RJV, de Souza CAF, de Souza JI, Dentinger BTM, Dissanayake
AJ, Doilom M, Drechsler-Santos ER, Ghobad-Nejhad M,
Gilmore SP, Góes-Neto A, Gorczak M, Haitjema GH, Hapuarachchi KK, Hashimoto A, He MQ, Henske JK, Hirayama K,
Iribarren MJ, Jayasiri SC, Jayawardena RS, Jeon SJ, Jerónimo
GH, Jesus AL, Jones EBG, Kang JC, Karunarathna SC, Kirk PM,
Konta S, Kuhnert E, Langer E, Lee HS, Lee HB, Li WJ, Li XH,
Liimatainen K, Lima DX, Lin CG, Liu JK, Liu XZ, Liu ZY,
Luangsa-ard JJ, Lücking R, Lumbsch HT, Lumyong S, Leaño
EM, Marano AV, Matsumura M, McKenzie EHC, Mongkolsamrit S, Mortimer PE, Nguyen TTT, Niskanen T,
123
76
Norphanphoun C, O’Malley MA, Parnmen S, Pawłowska J,
Perera RH, Phookamsak R, Phukhamsakda C, Pires-Zottarelli
CLA, Raspé O, Reck MA, Rocha SCO, de Santiago ALCMA,
Senanayake IC, Setti L, Shang QJ, Singh SK, Sir EB, Solomon
KV, Song J, Srikitikulchai P, Stadler M, Suetrong S, Takahashi
H, Takahashi T, Tanaka K, Tang LP, Thambugala KM,
Thanakitpipattana D, Theodorou MK, Thongbai B, Thummarukcharoen T, Tian Q, Tibpromma S, Verbeken A, Vizzini
A, Vlasák J, Voigt K, Wanasinghe DN, Wang Y, Weerakoon G,
Wen HA, Wen TC, Wijayawardene NN, Wongkanoun S,
Wrzosek M, Xiao YP, Xu JC, Yan JY, Yang J, Yang SD, Hu
Y, Zhang JF, Zhao J, Zhou LW, Peršoh D, Phillips AJL,
Maharachchikumbura SSN (2016) Fungal divers notes 253–366:
taxonomic and phylogenetic contributions to fungal taxa. Fungal
Divers 78:1–237
Li WJ, Bhat DJ, Camporesi E, Tian Q, Wijayawardene NN, Dai DQ,
Phookamsak R, Chomnunti P, Bahkali AH, Hyde KD (2015)
New asexual morph taxa in Phaeosphaeriaceae. Mycosphere
6:681–708
Liang C, Jayawardena RS, Zhang W, Wang X, Liu M, Liu L, Zang C,
Xu X, Hyde KD, Yan J, Li X, Zhao K (2016) Identification and
characterization of Pseudocercospora species causing grapevine
leaf spot in China. J Phytopathol 164:75–85
Linaldeddu BT, Deidda A, Scanu B, Franceschini A, Serra S, BerrafTebbal A, Zouaoui Boutiti M, Ben Jamaa ML, Philips AJL
(2015) Diversity of Botryosphaeriaceae species associated with
grapevine and other woody hosts in Italy, Algeria and Tunisia,
with descriptions of Lasiodiplodia exigua and Lasiodiplodia
mediterranea sp. nov. Fungal Divers 71:201–214
Linaldeddu BT, Deidda A, Scanu B, Franceschini A, Alves A,
Abdollahzadeh J, Phillips AJL (2016) Phylogeny, morphology
and pathogenicity of Botryosphaeriaceae, Diatrypaceae and
Gnomoniaceae associated with branch diseases of hazelnut in
Sardinia (Italy). Eur J Plant Pathol 146:259–279
Litzenberger SC, Farr ML, Lip HT (1962) A preliminary list of
Cambodian plant diseases. Div Agric Nat Res, USAID Minist
Agric Phnom-Penh, Cambodia
Liu PSW (1977) A supplement to a host list of plant diseases in
Sabah, Malaysia. Phytopathol Pap 21:1–49
Liu X-J, Guo Y-L (eds) (1998) Flora Fungorum Sinicorum. Pseudocercospora, vol 9. Science Press, Beijing
Liu JK, Hyde KD, Jones EBG, Ariyawansa HA, Bhat DJ, Boonmee S,
Maharachchikumbura S, McKenzie EHC, Phookamsak R,
Phukhamsakda C, Shenoy BD, Abdel-Wahab MA, Buyck B,
Chen J, Chethana KWT, Singtripop C, Dai DQ, Dai YC,
Daranagama DA, Dissanayake AJ, Doliom M, D’souza MJ, Fan
XL, Goonasekara ID, Hirayama K, Hongsanan S, Jayasiri SC,
Jayawardena RS, Karunarathna SC, Li WJ, Mapook A, Norphanphoun C, Pang KL, Perera RH, Peršoh D, Pinruan U,
Senanayake IC, Somrithipol S, Suetrong S, Tanaka K, Thambugala KM, Tian Q, Tibpromma S, Udayanga D, Wijayawardena
NN, Wanasinghe D, Wisitrassameewong K, Abdel-Aziz FA,
Adamčı́k S, Bahkali AH, Boonyuen N, Bulgakov T, Callac P,
Chomnunti P, Greiner K, Hashimoto A, Hofstetter V, Kang JC,
Lewis D, Li XH, Liu XX, Liu ZY, Matumura M, Mortimer PE,
Rambold G, Randrianjohany E, Sato G, Sri-Indrasutdhi V, Tian
CM, Verbeken A, von Brackel W, Wang Y, Wen TC, Xu JC,
Yan JY, Zhao RL, Camporesi E (2015) Fungal diversity notes
1–110: taxonomic and phylogenetic contributions to fungal
species. Fungal Divers 72:1–197
Liu QL, Li GQ, Li JQ, Chen SF (2016a) Botrytis eucalypti, a novel
species isolated from diseased Eucalyptus seedlings in South
China. Mycol Progr 15:1057–1079
Liu M, Zhang W, Zhou Y, Liu Y, Yan JY, Li XH, Jayawardena RS,
Hyde KD (2016b) First report of twig anthracnose on grapevine
123
Fungal Diversity (2018) 90:1–84
caused by Colletotrichum nymphaeae in China. Plant Dis
100:2530
Lombard L, Houbraken J, Decock C, Samson RA, Meijer M, Réblová
M, Groenewald JZ, Crous PW (2016) Generic hyper-diversity in
Stachybotriaceae. Persoonia 36:156
Longland JM, Sutton TB (2008) Factors affecting the infection of
fruit of Vitis vinifera by the bitter rot pathogen Greeneria
uvicola. Phytopathology 98:580–584
Lorsuwan C, Tontyaporn S, Visarathanonth N, Manoch L, Kakishima
M (1984) Materials for the rust flora in Thailand I. Trans Mycol
Soc Jpn 25:57–65
Lotz-Winter H, Hofmann T, Kirschner R, Kursawe M, Trampe T,
Piepenbring M (2011) Fungi in the Botanical Garden of the
University of Frankfurt. Z Mykol 77:89–122
Lu B, Hyde KD, Ho WH, Tsui KM, Taylor JE, Wong KM, Yanna,
Zhou D (2000) Checklist of Hong Kong Fungi. Fungal Diversity
Press, Hong Kong
Lubbe CM, Denman S, Cannon PF, Groenewald JZ, Lamprecht SC,
Crous PW (2004) Characterization of Colletotrichum species
associated with diseases of Proteaceae. Mycologia
96:1268–1279
Lücking R, Moncada B (2017) Dismantling Marchandiomphalina
into Agonimia (Verrucariaceae) and Lawreymyces gen. nov.
(Corticiaceae): setting a precedent to the formal recognition of
thousands of voucherless fungi based on type sequences. Fungal
Divers 84:119–138
Luongo L, Santori A, Riccioni L, Belisario A (2011) Phomopsis sp.
associated with post-harvest fruit rot of kiwifruit in Italy. J Plant
Pathol 93:205–209
Luque J, Martos S, Phillips AJL (2005) Botryosphaeria viticola sp.
nov. on grapevines: a new species with a Dothiorella anamorph.
Mycologia 97:1111–1121
Luque J, Martos S, Aroca A, Raposo R, Garcia-Figueres F (2009)
Symptoms and fungi associated with declining mature grapevine
plants in northeast Spain. J Plant Pathol 91:381–390
Magoč T, Salzberg SL (2011) FLASH: fast length adjustment of short
reads to improve genome assemblies. Bioinformatics
27:2957–2963
Magyar D, Shoemaker RA, Bobvos J, Crous PW, Groenewald JZ
(2011) Pyrigemmula, a novel hyphomycete genus on grapevine
and tree bark. Mycol Progr 10:307–314
Maharachchikumbura SSN, Guo LD, Chukeatirote E, Bahkali AH,
Hyde KD (2011) Pestalotiopsis—morpholgy, phylogeny,
biochemsitry and diversity. Fungal Divers 50:167–187
Maharachchikumbura SSN, Crous PW, Groenewald JZ, Xu J, Hyde
KD (2014) Pestalotiopsis revisited. Stud Mycol 79:121–186
Maharachchikumbura SN, Hyde KD, Jones EBG, McKenzie EHC,
Huang SK, Abdel-Wahab MA, Daranagama DA, Dayarathne M,
D’souza MJ, Goonasekara ID, Hongsanan S, Jayawardena RS,
Kirk PM, Konta S, Liu JK, Liu Z-Y, Norphanphoun C, Pang KL,
Perera RH, Senanayake IC, Shang Q, Shenoy BD, Xiao Y,
Bahkali AH, Kang J, Somrothipol S, Suetrong S, Wen T, Xu J
(2015) Towards a natural classification and backbone tree for
Sordariomycetes. Fungal Divers 72:199
Maharachchikumbura SSN, Larigon P, Hyde KD, Al-Sadi AM, Liu Z
(2016) Characteriztion of Neopestalotiopsis, Pestalotiopsis and
Truncatella species associated with grapevine trunk disease in
France. Phytopathol Mediterr 55:380–390
Mahdian S, Zafari D (2017) First report of table grape blue mold
caused by Penicillium sumatrense in Iran. Plant Dis 101:244
Makovetz S (1933) Contributions to the mycoflora of the Ukraine.
Bull Jard Bot Kieff 16:71–87
Maluta D-R, Larignon P (1991) Pied-noir: mieux vaut prévenir.
Viticulture 11:71–72
Fungal Diversity (2018) 90:1–84
Manamgoda DS, Rossman AY, Castlebury LA, Crous PW, Madrid H,
Chukeatirote E, Hyde KD (2014) The genus Bipolaris. Stud
Mycol 79:221–288
Maneval WE (1937) A list of the Missouri Fungi; with special
reference to plant pathogens and wood-destroying species. Univ
Missouri Stud Sci Ser 12:1–150
Marais PG (1979) Fungi associated with root rot in vineyards in the
Western Cape. Phytophylactica 11:65–68
Marais PG (1980) Fungi associated with decline and death of nursery
grapevines in the Western Cape. Phytophylactica 12:9–13
Marchesi JR, Ravel J (2015) The vocabulary of microbiome research:
a proposal. Microbiome 3:31
Marin-Felix Y, Groenewald JZ, Cai L, Chen Q, Marincowitz S,
Barnes I, Bensch K, Braun U, Camporesi E, Damm U, de Beer
ZW, Dissanayake A, Edwards J, Giraldo A, Hernández-Restrepo
M, Hyde KD, Jayawardena RS, Lombard L, Luangsa-ard J,
McTaggart AR, Rossman AY, Sandoval-Denis M, Shen M,
Shivas RG, Tan YP, van der Linde EJ, Wingfield MJ, Wood AR,
Zhang JQ, Zhang Y, Crous PW (2017) Genera of phytopathogenic fungi: GOPHY 1. Stud Mycol 86:99–216
Martin MT, Cobos R (2007) Identification of fungi associated with
grapevine decline in Castilla y Leon (Spain). Phytopathol
Mediterr 46:18–25
Martin MT, Martin L, de-Francisco MT, Cobos R (2009) First report
of Lasiodiplodia theobromae and Cryptovalsa ampelina associated with grapevine decline from Castilla y Leon, Spain. Plant
Dis 93:545
Martin MT, Martin L, Cuesta MJ, Garcia-Benavides P (2011a) First
report of Cylindrocarpon pauciseptatum associated with grapevine decline from Castilla y Leon, Spain. Plant Dis 95:361
Martin MT, Martin L, Cuesta MJ (2011b) First report of Neofusicoccum mediterraneum and N. austral causing decay in Vitis
vinifera in Castilla y Leon, Spain. Plant Dis 95:876
Martin FN, Blair JE, Coffey MD (2014) A combined mitochondrial
and nuclear multilocus phylogeny of the genus Phytophthora.
Fungal Genet Biol 66:19–32
Martiny JBH, Bohannan BJM, Brown JH, Colwell RK, Fuhrman JA,
Green JL, Horner-Devine MC, Kane M, Krumins JA, Kuske CR,
Morin PJ, Naeem S, Ovreås L, Reysenbach AL, Smith VH,
Staley JT (2006) Microbial biogeography: putting microorganisms on the map. Nat Rev Microbiol 4:102–112
Mathur RS (1979) The Coelomycetes of India. Bishen Singh
Mahendra Pal Singh, Delhi
Mayorquin JS, Wang DH, Twizeyimana M, Eskalen A (2016)
Identification, distribution, and pathogenicity of Diatrypaceae
and Botryosphaeriaceae associated with citrus branch canker in
the Southern California desert. Plant Dis 100:2402–2413
McDonald V, Eskalen A (2011) Botrysphaeriaceae species associated
with avacado branch cankers in California. Plant Dis
95:1465–1473
McKirdy SJ, Riley IT, Cameron IJ (1999) First report of grapevine
downy mildew (Plasmopara viticola) in commercial viticulture
in Western Australia. Plant Dis 83:301
McLeod A, Botha WJ, Meitz JC, Spies CFJ, Tewoldemedhin YT,
Mostert L (2009) Morphological and phylogenetic analyses of
Pythium species in South Africa. Mycol Res 113:933–951
Melnik VA, Popushoi IS (1992) Imperfect fungi on species of trees
and shrubs (U.S.S.R.). Unknown journal or publisher
Mena-Portales J, Delgado-Rodriguez G, Heredia-Abarca G (2000)
New combinations for species of Sporidesmium s.l. Bol Soc
Micol Madrid 25:265–269
Mendes MAS, da Silva VL, Dianese JC, Ferreira M, Santos CD,
Gomes NE, Urben A, Castro C (1998) Fungos em Plantas no
Brasil. Embrapa-SPI/Embrapa-Cenargen, Brasilia
Mey G, Oeser B, Lebrun MH, Tudzynski P (2002) The biotrophic,
non-appressorium-forming grass pathogen Claviceps purpurea
77
needs a Fus3/Pmk1 homologous mitogen-activated protein
kinase for colonization of rye ovarian tissue. Mol Plant Microbe
Interact 15:303–312
Michailides TJ, Peacock W, Christensen P, Morgan DP, Felts D
(2002) First report of Aspergillus vine canker of table grapes
caused by Aspergillus niger. Plant Dis 86:75
Milholland RD (1994) Macrophoma rot. In: Pearson RC, Goheen AC
(eds) Compendium of grape diseases. APS Press, St Paul
Miller JW (1991) Bureau of Plant Pathology. Tri-ol Tech Rep Div Pl
Ind Florida 30:2–4
Mills SD, Foerster H, Coffey MD (1991) Taxonomic structure of
Phytophthora cryptogea and P. drechsleri based on isozyme and
mitochondrial DNA analyses. Mycol Res 95:31–48
Mirzaei S, Nahvi MJ, Khaledi E, Abdollahzadeh J, Amini J,
Abrinbana M (2015) Molecular and morphological characterization of Endoconidioma populi from Kurdistan province, Iran.
Mycol Iran 2:127–133
Mitchell JI, Zuccaro A (2006) Sequences, the environment and fungi.
Mycologist 20:62–74
Mohammadi H, Banihashemi Z (2012) First report of Phaeoacremonium inflatipes and Phaeoacremonium mortoniae associated
with grapevine Petri disease in Iran. J Agric Sci Technol
14:1405–1414
Mohammadi H, Banihashemi Z, Gramaje D, Armengol J (2013a)
Fungal pathogens associated with grapevine trunk diseases in
Iran. J Agric Sci Technol 15:137–150
Mohammadi H, Gramaje D, Banihashemi Z, Armengol J (2013b)
Characterization of Diplodia seriata and Neofusicoccum parvum
associated with grapevine decline in Iran. J Agric Sci Technol
15:603–616
Moller WJ, Kasimatis AN, Kissler JJ (1974) A dying arm disease of
grape in California. Plant Dis Rep 58:869–871
Mondello V, Lo Piccolo S, Conigliaro G, Alfonzo A, Torta L,
Burruano S (2013) First report of Neofusicoccum vitifusiforme
and presence of the Botryosphaeriaceae species associated with
Botryosphaeria dieback of grapevine in Sicily (Italy). Phytopathol Mediterr 52:388–396
Montagne JFC (1856) Sylloge generum specierumque plantarum
cryptogamarum, vol 1. J. B. Bailliere, Paris, pp. 1–498
Moralejo E, Clemente A, Descals E, Belbahri L, Calmin G, Lefort F,
Spies CFJ, McLeod A (2008) Pythium recalcitrans sp. nov.
revealed by multigene phylogenetic analysis. Mycologia
100:310–319
Morgan DP, Michailides TJ (2004) First report of melting decay of
‘Red Globe’ grapes in California. Plant Dis 88:1047
Mostert L, Crous PW, Kang JC, Phillips AJL (2001) Species of
Phomopsis and a Libertella sp. occurring on grapevines with
specific reference to South Africa: morphological, cultural,
molecular and pathological characterization. Mycologia
93:146–167
Mostert L, Halleen F, Creaser ML, Crous PW (2004) Cryptovalsa
ampelina, a forgotten shoot and cane pathogen of grapevines.
Australas Plant Pathol 33:295–299
Mostert L, Halleen F, Fourie P, Crous PW (2006) A review of
Phaeoacremonium species involved in Petri disease and esca of
grapevines. Phytopathol Mediterr 45:12–29
Mouchacca J (2009) Novel fungal taxa from the arid Middle East
introduced prior to the year 1940. II. Anamorphic fungi:
hypomycetes. Cryptog Mycol 30:199–222
Mugnai L, Graniti A, Surico G (1999) Esca (black measles) and
brown wood-streaking: two old and elusive diseases of grapevines. Plant Dis 83:404–418
Mujica F, Oehrens B (1967) Segunda addenda a flora fungosa
Chilena. Boletin Tecnico 27:1–78
123
78
Mujica F, Vergara C (1945) Flora fungosa Chilena. Indice preliminar
de los huespedes de los hongos chilenos y sus referencias
bibliograficas. Imprenta Stanley
Mulenko W, Majewski T, Ruszkiewicz-Michalska M (2008) A
preliminary checklist of micromycetes in Poland, vol 9.
W. Szafer Institute of Botany, Polish Academy of Sciences,
p 752
Mundkur BB (1943) Indian species of Phakopsora and Bubakia.
Mycologia 35:538–545
Mundkur BB, Thirumalachar MJ (1946) Revisions of and additions to
Indian fungi. I. Mycol Pap 16:1–27
Muthumary J, Qaiser AS, Sutton BC (1986) Reassessment of
Monochaetia terminaliae. Trans Br Mycol Soc 87:103–108
Nag Raj TR (1988) Redisposals and redescriptions in the Monochaetia-Seiridium, Pestalotia-Pestalotiopsis complexes. VIII.
On the status of Monochaetia camelliae, M. osyridella and
Pestalotia gaurae. Mycotaxon 32:121–132
Nag Raj TR (1993) Coelomycetous anamorphs with appendagebearing conidia. Mycologue Publications, Waterloo, pp 1–1101
Nag Raj TR, Kendrick B (1975) A monograph of Chalara and allied
genera. Wilfrid Laurier University Press, Ontario
Nagorny P (1930) Die pilsflora der Kaukasischen Weinreve. Trav Jard
Bot Tiflis Ser II 5:1–201
Nakagiri A, Tadayoshi ITO, Hatamoto M (1994) Brown zonate spot
of grape caused by Briosia ampelophaga. Jpn J Phytopathol
60:608–612
Nakaune R, Tatsuki M, Matsumoto H, Ikoma Y (2016) First report of
a new postharvest disease of grape caused by Cadophora luteoolivacea. J Gen Plant Pathol 82:116–119
Nasyrov O (1964) Some species of fungi Imperfecti, new for
Turkmenistan in the valley of the middle Ama-Darya. Akad
Nauk Turkmen SSR Iav Ser Biol Nauk 3:1–116
Nattrass RM (1961) Host lists of Kenya fungi and bacteria. Mycol
Pap 81:1–46
Navarrete F, Abreo E, Bettucci L, Martinez S, Lupo S (2009) First
report of Greeneria uvicola as cause of grapevine dead-arm
dieback in Uruguay. Australas Plant Dis Notes 4:117–119
Netto MSB, Assuncao IP, Lima GSA, Marques MW, Lima WG,
Monteiro JHA, Michereff SJ, Phillips AJL, Camara MPS, de
Queiroz Balbino V (2014) Species of Lasiodiplodia associated
with papaya stem-end rot in Brazil. Fungal Divers 67:127–141
Netto MSB, Lima WG, Correia KC, Da Silva CFB, Thon M, Martins
RB, Miller RNG, Michereff SJ, Camara MPS (2017) Analysis of
phylogeny, distribution, and pathogenicity of Botryosphaeriaceae species associated with gummosis of Anacardium in
Brazil, with a new species of Lasiodiplodia. Fungal Biol
121:437–451
Nguyen NH, Song Z, Bates ST, Branco S, Tedersoo L, Menke J,
Schilling JS, Kennedy PG (2015) FUNGuild: an open annotation
tool for parsing fungal community datasets by ecological guild.
Fungal Ecol 20:241–248
Niessl G (1871) Beiträge zur Kenntniss der Pilze. Beschreibung neuer
und wenig bekannter Pilze. Verhandlungen des Naturforschenden Vereines in Brünn 10:153–217
Nogueira AF Jr, Fischer IH, Braganca CAD, Massola NS Jr, Amorim
L (2016) Identification of Botryosphaeriaceae species that cause
stylar-end rot of guavas and characterisation of the disease
monocycle. Eur J Plant Pathol 144:271–287
Nomura Y, Takamatsu S, Fujioka K (2003) Teleomorph of Erysiphe
necator var. necator on Vitis vinifera and Ampelopsis brevipedunculata var. heterophylla (Vitaceae) newly found in
Japan. Mycoscience 44:157–158
Norse D (1974) Plant diseases in Barbados. Phytopathol Pap 18:1–38
O’Donnell K, Cigelnik E, Nirenberg HI (1998) Molecular systematics
and phylogeography of the Gibberella fujikuroi species complex.
Mycologia 90:465–493
123
Fungal Diversity (2018) 90:1–84
Oh S-Y, Nam K-W, Yoon D-H (2014) Identification of Acremonium
acutatum and Trichothecium roseum isolated from grape with
white stain symptom in Korea. Mycobiology 42:269–273
Ono Y (2000) Taxonomy of the Phakopsora ampelopsidis species
complex on vitaceous hosts in Asia includes a new species, P.
euvitis. Mycologia 92:154–173
Ono Y (2016) Mixed infections of grapevine leaf rusts Phakopsora
meliosmae-myrianthae and P. montana in Japan. J Gen Plant
Pathol 82:149–153
Orieux L, Felix S (1968) List of plant diseases in Mauritius.
Phytopathol Pap 7:1–48
Oudemans P, Coffey MD (1991) Isozyme comparison within and
among worldwide sources of three morphologically distinct
species of Phytophthora. Mycol Res 95:19–30
Ozben S, Demirci F, Degirmenci K, Uzunok S (2012) First report of
Cylindrocarpon macrodidymum associated with black foot
diseases of Grapevine in Turkey. Plant Dis 96:762
Padwick GW (1946) Notes on Indian fungi. IV. Mycol Pap 17:1–12
Pan FY, Huang Y, Lin L, Zhou YM, Wei RF, Guo WF, Yin L, Lu J
(2016) First report of Colletotrichum capsici causing grape ripe
rot in Guangxi, China. Plant Dis 100:2531
Pancher M, Ceol M, Corneo PE, Longa CMO, Yousaf S, Pertot I,
Campisano A (2012) Fungal endophytic communities in
grapevines (Vitis vinifera L.) respond to crop management.
Appl Environ Microbiol 78:4308–4317
Pande A (2008) Ascomycetes of Peninsular India. Scientific Publishers (India), Jodhpur
Pantidou ME (1973) Fungus–host index for Greece. Benaki Phytopathological Institute, Kiphissia, Athens
Paolinelli-Alfonso M, Villalobos-Escobedo JM, Rolshausen P, Herrera-Estrella A, Galindo-Sánchez C, López-Hernández JF,
Hernandez-Martinez R (2016) Global transcriptional analysis
suggests Lasiodiplodia theobromae pathogenicity factors
involved in modulation of grapevine defensive response. BMC
Genomics 17:615
Pardo Cardona VM (1998) Distribucion de las especies colombianas
de Uredinales segun los grupos taxonomicos de sus hospederos.
Rev Fac Nal Agr Medellin 51:285–319
Park M-J, Choi Y-J, Hong S-B, Shin H-D (2010) Genetic variability
and mycohost association of Ampelomyces quisqualis isolates
inferred from phylogenetic analyses of ITS rDNA and actin gene
sequences. Fungal Biol 114:235–247
Parkinson LE, Shivas RG, Dann EK (2017) Pathogenicity of
Nectriaceous fungi on avocado in Australia. Phytopathology
107:1479–1485
Parris GK (1959) A revised host index of Mississippi plant diseases.
Miss State Univ Bot Dept Misc Publ 1:1–146
Pascoe I, Cottral E (2000) Developments in grapevine trunk diseases
research in Australia. Phytopathol Mediterr 39:68–75
Passerini (1872) Erb Critt Ital Ser 2:595
Patil MS, Mahamulkar SH (1999) Studies on Meliolaceae of India IV.
Indian Phytopathol 52:245–253
Paul YS, Thakur VK (2006) Indian Erysiphaceae. Scientific Publishers (India), Jodhpur
Pavlic-Zupanc D, Piskur B, Slippers B, Wingfield MJ, Jurc D (2015)
Molecular and morphological characterization of Dothiorella
species associated with dieback of Ostrya carpinifolia in
Slovenia and Italy. Phytopathol Mediterr 54:222–231
Pearson RC, Smith FD, Dubos B (1988) Angular leaf scorch, a new
disease of grapevines in North America caused by Pseudopezicula tetraspora. Plant Dis 72:796–800
Peng L-J, Sun T, Yang Y-L, Cai L, Hyde KD, Bahkali AH, Liu Z-Y
(2013) Colletotrichum species on grape in Guizhou and Yunnan
provinces, China. Mycoscience 54:29–41
Pennycook SR (1989) Plant diseases recorded in New Zealand, vols
1–3. Plant Diseases Division, DSIR, Auckland
Fungal Diversity (2018) 90:1–84
Peregrine WTH, Ahmad KB (1982) Brunei: a first annotated list of
plant diseases and associated organisms. Phytopathol Pap
27:1–87
Peregrine WTH, Siddiqi MA (1972) A revised and annotated list of
plant diseases in Malawi. Phytopathol Pap 16:1–51
Péros JP, Jamaux-Despréaux I, Berger G, Gerba D (1999) The
potential importance of diversity in Eutypa lata and cocolonising fungi in explaining variation in development of
grapevine dieback. Mycol Res 103:1385–1390
Peter G, Tornai-Lehoczki J, Suzuki M, Dlauchy D (2005) Metschnikowia viticola sp. nov., a new yeast species from grape. Antonie
van Leeuwenhoek Suppl 87:155–160
Petit E, Gubler WD (2005) Characterization of Cylindrocarpon
species, the cause of black foot disease of grapevine in
California. Plant Dis 89:1051–1059
Petit E, Gubler WD (2007) First report of Cylindrocarpon liriodendri
causing black foot disease of grapevine in California. Plant Dis
91:1060
Petit E, Barriault E, Baumgartner K, Wilcox WF, Rolshausen PE
(2011) Cylindrocarpon species associated with black-foot of
grapevine in northeastern United States and southeastern
Canada. Am J Enol Vitic 62:177–183
Petrak F (1953) Ein Beitrag zur Pilzflora Floridas. Sydowia
7:103–116
Petrak F, Sydow H (1927) Die Gattungen der Pyrenomyzeten,
Sphaeropsideen und Melanconieen. 1. Die phaeosporen
Sphaeropsideen und die Gattung Macrophoma. Repert Spec
Nov Regni Veg 42:1–551
Petrini LE (1992) Rosellinia species of the temperate zones. Sydowia
44:169–281
Petrini LE (2013) Rosellinia—a world monograph. Biblioth Mycol
205:410
Pettersson OV, Leong SL, Lantz H, Rice T, Dijksterhuis J, Houbraken
J, Samson RA, Schnurer J (2011) Phylogeny and intraspecific
variation of the extreme xerophile, Xeromyces bisporus. Fungal
Biol 115:1100–1111
Phengsintham P, Braun U, McKenzie EHC, Chukeatirote E, Cai L,
Hyde KD (2013) Monograph of Cercosporoid fungi from
Thailand. Plant Pathol Q 3:67–138
Phillips AJL (1998) Botryosphaeria dothidea and other fungi
associated with excoriose and dieback of grapevines in Portugal.
J Phytopathol 146:327–332
Phillips AJL (1999) The relationship between Diaporthe perjuncta
and Phomopsis viticola on grapevines. Mycologia 91:1001–1007
Phillips AJL (2000) Excoriose, cane blight and related diseases of
grapevines: a taxonomic review of the pathogens. Phytopathol
Mediterr 39:341–356
Phillips AJL, Lucas MT (1997) The taxonomic status of Macrophoma
flaccid and Macrophoma reniformis and their relationship to
Botryosphaeria dothidea. Sydowia 49:150–159
Phillips AJL, Fonseca F, Povoa V, Castilho R, Nolasco G (2002) A
reassessement of the anamorphic fungus Fusicoccum luteum and
description of its teleomorph Botryosphaeria lutea sp. nov.
Sydowia 54:59–77
Phillips A, Alves A, Correia A, Luque J (2005) Two new species of
Botryosphaeria with brown, 1-septate ascospores and Dothiorella anamorphs. Mycologia 97:513–529
Pintos Varela C, Redondo Fernandez V, Aguin Casal O, Ferreiroa
Martinez V, Mansilla Vazquez JP (2016) First report of
Pleurostoma richardsiae causing grapevine trunk disease in
Spain. Plant Dis 100:2168
Pintos VC, Redondo Fernandez V, Aguin Casal O, Mansilla Vazuez
JP (2011) First report of cankers and dieback caused by
Neofusicoccum mediterraneum and Diplodia corticola on
Grapevine in Spain. Plant Dis 95:1315
79
Piqueras CM, Herrera D, Latorre BA (2014) First report of high
boscalid resistance in Botrytis cinerea associated with the
H272L mutation in grapevine in Chile. Plant Dis 98:1441
Pirnia M, Zare R, Zamanizadeh HR, Khodaparast A (2012) New
records of cercosporoid hyphomycetes from Iran. Mycotaxon
120:157–169
Pitt WM, Huang R, Steel CC, Savocchia S (2010) Identification,
distribution and current taxonomy of Botryosphaeriaceae
species associated with grapevine decline in New South Wales
and South Australia. Aust J Grape Wine Res 16:258–271
Pitt WM, Úrbez-Torres JR, Trouillas FP (2013) Dothiorella vidmadera, a novel species from grapevines in Australia and notes
on Spencermartinsia. Fungal Divers 61:209–219
Pitt WM, Úrbez-Torres JR, Trouillas FP (2015) Dothiorella and
Spencermartinsia, new species and records from grapevines in
Australia. Australas Plant Pathol 44:43–56
Pollack FG (1987) An annotated compilation of Cercospora names.
Mycol Mem 12:1–212
Pons N, Sutton BC (1988) Cercospora and similar fungi on yams
(Dioscorea species). Mycol Pap 160:1–78
Pota S, Chatasiri S, Unartngam J, Yamaoka Y, Hosaka K, Ono Y
(2015) Taxonomic identity of a Phakopsora fungus causing the
grapevine leaf rust disease in Southeast Asia and Australasia.
Mycoscience 56:198–204
Preston DA (1945) Host index of Oklahoma plant diseases. Oklahoma
Agric Coll Agric Exp Sta Techn Bull T 21:1–168
Priest MJ (2006) Fungi of Australia: Septoria. ABRS/CSIRO
Publishing, Canberra/Melbourne
Prodorutti D, De Luca F, Michelon L, Pertot I (2009) Susceptibility to
Armillaria mellea root rot in grapevine rootstocks commonly
grafted onto Teroldego Rotaliano. Phytopathol Mediterr
48:285–290
Promputtha I, Lumyong S, Dhanasekaran V, McKenzie EHC, Hyde
KD, Jeewon R (2007) A phylogenetic evaluation of whether
endophytes become saprotrophs at host senescence. Microb Ecol
53:579–590
Promputtha I, Hyde KD, McKenzie EH, Peberdy JF, Lumyong S
(2010) Can leaf degrading enzymes provide evidence that
endophytic fungi becoming saprobes? Fungal Divers 41:89–99
Purahong W, Wubet T, Krüger D, Buscot F (2018) Molecular
evidence strongly supports deadwood-inhabiting fungi exhibiting unexpected tree species preferences in temperate forests.
ISME J 12:article 289
Qiu Y, Steel CC, Ash GJ, Savocchia S (2011) Survey of
Botryosphaeriaceae associated with grapevine decline in the
Hunter Valley and Mudgee grape growing regions of New South
Wales. Australas Plant Pathol 40:1–11
Raabe RD (1966) Check list of plant diseases previously unreported
in Hawaii. Plant Dis Rep 50:411–414
Raabe RD, Conners IL, Martinez AP (1981) Checklist of plant
diseases in Hawaii. College of Tropical Agriculture and Human
Resources, University of Hawaii. Information Text Series No.
22. Hawaii Inst Trop Agric Human Resources
Radulescu E, Negru A, Docea E (1973) Septoriozele din Romania. Ed
Acad Rep Soc Romania Bucarest
Ragunathan AN, Ramakrishnan K (1973) Rust fungi of Madras State.
VII. Kuehneola, Hamaspora, Phragmotelium, Phragmidium,
Diorchidium, Ravenelia, Hapalophragmium and Nyssopsora.
Mysore J Agric Sci 7:73–86
Raimondo ML, Lops F, Carlucci A (2014) Phaeoacremonium
italicum sp. nov., associated with esca of grapevine in southern
Italy. Mycologia 106:1119–1126
Rajak RC, Pandey AK (1985) Fungi from Jabalpur-II. Indian J Mycol
Plant Pathol 15:186–194
Rajchenberg M, Robledo G (2013) Pathogenic polypores in
Argentina. For Pathol 43:171–184
123
80
Rappaz F (1987) Taxonomy and nomenclature of the octosporous
Diatrypaceae. Mycol Helv 2:285–648
Rastogi G, Sani RK (2011) Molecular techniques to assess microbial
community structure, function, and dynamics in the environment. In: Microbes and microbial technology, Springer, New
York, pp29–57
Reddy MS, Reddy KRC (1983) Greeneria fruit rot—an endemic
disease of grape in India. Indian Phytopathol 36:110–114
Rego C, Oliveira H, Carvalho A, Phillips A (2000) Involvement of
Phaeoacremonium spp. and Cylindrocarpon destructans with
grapevine decline in Portugal. Phytopathol Mediterr 39:76–79
Riley EA (1960) A revised list of plant diseases in Tanganyika
Territory. Mycol Pap 75:1–42
Rolshausen PE, Trouillas F, Gubler WD (2004) Identification of
Eutypa lata by PCR-RFLP. Plant Dis 88:925–929
Rolshausen PE, Akgul DS, Perez R, Eskalen A, Gispert C (2013) First
report of wood canker caused by Neoscytalidium dimidiatum on
grapevine in California. Plant Dis 97:1511
Rolshausen PE, Baumgartner K, Travadon R, Pouzoulet J, Fujiyoshi
P, Wilcox WF (2014) Identification of Eutypa spp. causing
Eutypa dieback of grapvine in Eastern North America. Plant Dis
98:483–491
Rooney-Latham S, Janousek CN, Eskalen A, Gubler WD (2008) First
report of Aspergillus carbonarius causing Sour rot of
table grapes (Vitis vinifera) in California. Plant Dis 92:651
Roux J, Wingfield MJ, Morris MJ (1997) Botryosphaeria dothidea, a
pathogen of Acacia mearnsii in South Africa. S Afr J Sci 93:xii
Rusanov VA, Bulgakov TS (2008) Powdery mildew fungi of Rostov
region. Mikol Fitopatol 42:314–322
Ruszkiewicz-Michalska M, Michalski M (2005) Phytopathogenic
micromycetes in central Poland. I. Peronosporales and Erysiphales. Acta Mycol 40:223–250
Saccardo PA (1878) Fungi Veneti novi vel critici vel mycologiae
Venetae addendi. Ser VII Michelia 1:133–221
Saccardo P, Traverso G (1903) Contribuzione alla flora micologica
della Sardegna. Ann Myc 1:427–444
Saito S, Margosan D, Michailides TJ, Xiao CL (2016) Botrytis
californica, a new cryptic species in the B. cinerea species
complex causing gray mold in blueberries and table grapes.
Mycologia 108:330–343
Sakalidis ML, Slippers B, Wingfield BD, St J Hardy GE, Burgess TI
(2013) The challenge of understanding the origin, pathways and
extent of fungal invasions: global populations of the Neofusicoccum parvum—N. ribis species complex. Div Distrib
19:873–883
Salazar-Yepes M, Buritica P, Cadena-Gomez G (2002) Implicaciones
de los estudios sobre biodiversidad de los Uredinales (Royas) en
la region cafetera colombiana. Cenicafe 53:219–238
Sami S, Mohammadi H, Heydarnejad J (2014) Phaeoacremonium
species associated with necrotic wood of pome fruit trees in Iran.
J Plant Pathol 96:487–495
Sanoamuang N, Jitjak W, Rodtong S, Whalley AJS (2013) Gelatinomyces siamensis gen. sp. nov. (Ascomycota, Leotiomycetes,
incertae sedis) on bamboo in Thailand. IMA Fungus 4:71–87
Santos C, Fragoeiro S, Valentim H, Phillips A (2006) Phenotypic
characterisation of Phaeoacremonium and Phaeomoniella strains
isolated from grapevines: enzyme production and virulence of
extra-cellular filtrate on grapevine calluses. Sci Horti
107:123–130
Santos JM, Correia VG, Phillips AJL (2010) Primers for mating-type
diagnosis in Diaporthe and Phomopsis: their use in teleomorph
induction in vitro and biological species definition. Fungal Biol
114:255–270
Santos R, Blume E, Muniz M, Harakawa R, Garrido R, Rego C
(2014) Characterization of Campylocarpon pseudofasciculare
123
Fungal Diversity (2018) 90:1–84
associated with black foot of grapevine in southern Brazil.
Phytopathol Mediterr 53:06–415
Sarbhoy AK, Agarwal DK (1990) Descriptions of tropical plant
pathogenic fungi. Set 1 to 10. Malhotra Publ. House, New Delhi
Sarbhoy AK, Lal G, Varshney JL (1971) Fungi of India (1967–71).
Navyug Traders, New Delhi
Savas NG, Akgul DS, Albaz EA (2015) First report of Ilyonectria
liriodendra associated with black foot disease of grapevine in
Turkey. Plant Dis 99:1855
Savulescu T, Rayss T (1935) The species of Cercospora parasitic on
Vine leaves in Palestine. Rev Pathol Veg 22:3
Sawada K (1943) Descriptive catalogue of the Formosan fungi. Part
IX. Rep Dept Agric Govt Res Inst Formosa 86:1–178
Sawada K (1959) Descriptive catalogue of Taiwan (Formosan) fungi.
XI. Spec Publ Coll Agric Natl Taiwan Univ 8:1–268
Sawant IS, Narkar SP, Shetty DS, Upadhyay A, Sawant SD (2012)
First report of Colletotrichum capsici causing anthracnose on
grapes in Maharashtra, India. New Dis Rep 25:2
Scheck HJ, Vasquez SJ, Gubler WD (1998a) First report of black-foot
disease, caused by Cylindroncarpon obtusisporum, of grapevine
in California. Plant Dis 82:448
Scheck HJ, Vasquez SJ, Fogle D, Gubler WD (1998b) Grape growers
report losses to black-foot and grapevine decline. Calif Agric
52:19–23
Scheper RWA, Crane DC, Whisson DL, Scott ES (2000) The
Diaporthe teleomorph of Phomopsis taxon 1 on grapevine.
Mycol Res 104:226–231
Schoch CL, Seifert KA, Huhndorf S, Robert V, Spouge JL, Levesque
CA, Chen W (2012) Nuclear ribosomal internal transcribed
spacer (ITS) region as a universal DNA barcode marker for
Fungi. Proc Natl Acad Sci USA 109:6241–6246
Schubert K, Braun U (2005) Taxonomic revision of the genus
Cladosporium s.l. 4. Species reallocated to Asperisporium,
Dischloridium, Fusicladium, Passalora, Pseudoasperisporum
and Stenella. Fungal Divers 20:187–208
Schulzer S (1870) Mykologische Beiträge. Verhandlungen der
Zoologisch-Botanischen Gesellschaft Wien 20:635–658
Seifert KA (1985) A monograph of Stilbella and some allied
Hyphomycetes. Stud Mycol 27:1–234
Seifert KA, Axelrood PE (1998) Cylindrocarpon destructans var.
destructans. Can J Plant Pathol 20:115–117
Seifert KA, McMullen CR, Yee D, Reeleder RD, Dobinson KF
(2003) Molecular differentiation and detection of ginsengadapted isolates of the root rot fungus Cylindrocarpon destructans. Phytopathology 93:1533–1542
Seifert KA, Nickerson NL, Corlett M, Jackson ED, Louis-Seize G,
Davies RJ (2004) Devriesia, a new hyphomycete genus to
accommodate heat-resistant, Cladosporium-like fungi. Can J Bot
82:914–926
Senanayake IC, Maharachchikumbura SS, Hyde KD, Bhat JD, Jones
EG, McKenzie EH, Dai DQ, Daranagama DA, Dayarathne MC,
Goonasekara ID, Konta S, Li WJ, Shang QJ, Stadler M,
Wijayawardene NN, Xiao YP, Norphanphoun C, Li Q, Liu
XZ, Bahkali AH, Kang JC, Wang Y, Wen TC, Wendt L, Xu JC,
Camporesi E (2015) Towards unraveling relationships in Xylariomycetidae (Sordariomycetes). Fungal Divers 73:73–144
Sergeeva V, Priest M, Nair NG (2005) Preliminary studies on
Pestalotiopsis species from southern hemisphere conifers in
Australasia and South Africa. Australas Plant Pathol 34:255–258
Serra R, Peterson SW (2007) Penicillium astrolabium and Penicillium
neocrassum, two new species isolated from grapes and their
phylogenetic placement in the P. olsonii and P. brevicompactum
clade. Mycologia 99:78–87
Sessa L, Abreo E, Bettucci L, Lupo S (2016) Botryosphaeriaceae
species associated with wood diseases of stone and pome fruits
Fungal Diversity (2018) 90:1–84
trees: symptoms and virulence across different hosts in Uruguay.
Eur J Plant Pathol 146:519–530
Setati ME, Jacobson D, Bauer FF (2015) Sequence-based analysis of
the Vitis vinifera L. cv Cabernet Sauvignon grape must
mycobiome in three South African vineyards employing distinct
agronomic systems. Front microbial 6:article1358
Sharma HC, Agarwal DK (1997) A new anthracnose diseae of grape
vine (Vitis vinifera) in India. Indian Phytopathol 50:150
Shaw CG (1973) Host fungus index for the Pacific Northwest—I.
Hosts. Wash State Univ Agric Exp Sta Bull 765:1–121
Shi F, Hsiang T (2014) First Report of Pseudonectria buxi causing
Volutella Blight on Boxwood (Buxus sp.) in Beijing, China.
Plant Dis 98:1282–1282
Shirouzu T, Harada Y (2004) Notes on species of Helminthosporium
and its allied genera in Japan. Mycoscience 45:17–23
Shivas RG (1989) Fungal and bacterial diseases of plants in Western
Australia. J R Soc West Australia 72:1–62
Shivas RG, Tan YP, Edwards J, Dinh Q, Maxwell A, Andjic V,
Liberato JR, Anderson C, Beasley DR, Bransgrove K, Coates
LM, Cowan K, Daniel R, Dean JR, Lomavatu MF, MercadoEscueta D, Mitchell RW, Thangavel R, Tran-Nguyen LTT, Weir
BS (2016) Colletotrichum species in Australia. Australas Plant
Pathol 45:447–464
Shoemaker RA (1992) Catalogue of Pleospora names and types 1.
Alphabetically in hard copy and diskette 2. Sortable Data Base
on Diskette (available from the author or herb. BPI). Unknown
journal or publisher
Simmonds JH (1966) Host index of plant diseases in Queensland.
Queensland Department of Primary Industries, Brisbane
Simonyan SA (1981) Mycoflora of Botanical Gardens and Arboreta in
Armenia. Hayka
Slippers B, Smit WA, Crous PW, Coutinho TA, Wingfield BD,
Wingfield MJ (2007) Taxonomy, phylogeny and identification of
Botryosphaeriaceae associated with pome and stone fruit trees in
South Africa and other regions of the world. Plant Pathol
56:128–139
Smetham GM, Ades PK, Peros J-P, Ford R (2010) Genetic structure
of the grapevine fungal pathogen Phaeomoniella chlamydospora
in southeastern Australia and southern France. Plant Pathol
59:736–744
Sneath PH, Sokal RR (1973) Numerical taxonomy. The principles and
practice of numerical classification. Freeman WH, San Francisco
Sogonov MV, Castlebury LA, Rossman AY, Mejia LC, White JF
(2008) Leaf-inhabiting genera of the Gnomoniaceae, Diaporthales. Stud Mycol 62:1–79
Soliman EA, Abdel-Azeem AM, Salem FM, Nafady NA, Mehesien
MT, Ahmed AIS, Ibrahem ME, Abdel-Azeem MA, Hassan SS
(2016) A taxonomic analysis of fungi collected and described
from Egypt up to (1931). Stud Fungi 1:11–33
Sokal RR, Sneath PH (1963) Principles of numerical taxonomy. San
Francisco, p 359
Sosnowski MR, Lardner R, WicksTJ Scott ES (2007) The influence of
grapevine cultivar and isolate of Eutypa lata on wood and foliar
symptoms. Plant Dis 91:924–931
Sousa da Câmara M (1950) Catalogus Fungorum Juresi (Serra do
Gerês) ad Mycofloram Lusitanicam. Agron Lusit 12:89–122
Spegazzini (1878) Riv Viticolt Enolog Conegliano 2:727
Stevenson JA (1975) Fungi of Puerto Rico and the American Virgin
Islands. Contr Reed Herb 23:743
Stevenson JA, Wellman FL (1944) A preliminary account of the plant
diseases of El Salvador. J Wash Acad Sci 34:259–268
Stewart EJ (2012) Growing unculturable bacteria. J Bacteriol
194:4151–4160
Stoykov DY (2012) Diaporthales. Fungi Bulga 8:319
Stoykow DY, Denchev CM (2006) Current knowledge of Diaporthales (Ascomycota) in Bulgaria. Mycol Balcan 3:179–185
81
Sultan A, Johnston PR, Park D, Robertson AW (2011) Two new
pathogenic ascomycetes in Guignardia and Rosenscheldiella on
New Zealand’s pygmy mistletoes (Korthalsella: Viscaceae).
Stud Mycol 68:237–247
Sumstine DR (1949) The Albert Commons collection of fungi in the
herbarium of the Academy of Natural Sciences in Philadelphia.
Mycologia 41:11–23
Sutton BC (1969) Type studies of Coniella, Anthasthoopa, and
Cyclodomella. Can J Bot 47:603–608
Sutton BC (1975) Coelomycetes. V. Coryneum. Mycol Pap
138:1–224
Sutton BC (1980) The Coelomycetes. Fungi Imperfecti with Pycnidia,
Acervuli and Stromata. Commonwealth Mycological Institute,
Kew, Surrey
Suzuki MT, Giovannoni SJ (1996) Bias caused by template annealing
in the amplification of mixtures of 16S rRNA genes by PCR.
Appl Environ Microbiol 62:625–630
Swett CL, Bourret T, Gubler WD (2016) Characterizing the brown
spot pathosystem in late-harvest table grapes (Vitis vinifera L.) in
the California Central Valley. Plant Dis 100:2204–2210
Tai FL (1979) Sylloge Fungorum Sinicorum. Sci Press, Acad Sin
Peking, pp1527
Tanaka K, Harada Y (2003) Pleosporales in Japan (2): the genus
Lophiotrema. Mycoscience 44:115–121
Tao WC, Zhang W, Yan JY, Hyde KD, McKenzie EH, Li XH, Wang
Y (2014) A new Alternaria species from grapevine in China.
Mycol Prog 13:999
Tassi F (1902) I generi Phyllosticta Pers., Phoma Fr., Macrophoma
(Sacc.) Berl. & Voglino e i loro generi analoghi, giusta la legge
d’analogia. Bollettino del Laboratorio de Orto Botanico Reale
Universita Siena 5:1–76
Tatagiba SD, DaMatta FM, Rodrigues FÁ (2015) Leaf gas exchange
and chlorophyll a fluorescence imaging of rice leaves infected
with Monographella albescens. Phytopathology 105:180–188
Taylor A, St J Hardy GE, Wood P, Burgess T (2005) Identification
and pathogenicity of Botryosphaeria species associated with
grapevine decline in Western Australia. Australas Plant Pathol
34:187–195
Taylor DL, Walters WA, Lennon NJ, Bochicchio J, Krohn A,
Caporaso JG, Pennanen T (2016) Accurate estimation of fungal
diversity and abundance through improved lineage-specific
primers optimized for Illumina amplicon sequencing. Appl
Environ Microbiol 82:7217–7226
Tejesvi MV, Ruotsalainen AL, Markkola AM, Pirttilä AM (2010)
Root endophytes along a primary succession gradient in northern
Finland. Fungal Divers 41:125–134
Teng SC (1996) Fungi of China. Mycotaxon Ltd, Ithaca
Teodoro NG (1937) An Enumeration of Philippine Fungi. Tech Bull
Dept Agric Comm Manila 4:1–585
Terral JF, Tabard E, Bouby L, Ivorra S, Pastor T, Figueiral I, Picq S,
Chevance JB, Jung C, Fabre L, Tardy C (2009) Evolution and
history of grapevine (Vitis vinifera) under domestication: new
morphometric perspectives to understand seed domestication
syndrome and reveal origins of ancient European cultivars. Ann
Bot 105:443–455
Thaung MM (1984) Some fungi of Cercospora complex from Burma.
Mycotaxon 19:425–452
Thaung MM (2008a) Pathologic and taxonomic analysis of leaf spot
and tar spot diseases in a tropical dry to wet monsoon ecosystem
of lowland Burma. Australas Plant Pathol 37:180–197
Thaung MM (2008b) Report: some noteworthy fungi of Burma.
Australas Mycol 27:111–116
Thaung MM (2008c) Biodiversity survey of coelomycetes in Burma.
Australas Mycol 27:74–110
Tibpromma S, Hyde KD, Jeewon R, Maharachchikumbura SSN, Liu
JK, Bhat DJ, Jones EBG, McKenzie EHC, Camporesi E,
123
82
Bulgakov TS, Doilom M, ALCMA Santiago, Das K, Manimohan P, Gibertoni TB, Lim YW, Ekanayaka AH, Thongbai B, Lee
HB, Yang JB, Kirk PM, Sysouphanthong P, Singh SK, Boonmee
S, Dong W, Raj KNA, Latha KPD, Phookamsak R, Phukhamsakda C, Konta S, Jayasiri SC, Norphanphoun C, Tennakoon DS,
Li J, Dayarathne MC, Perera RH, Xiao Y, Wanasinghe DN,
Senanayake IC, Goonasekara ID, de Silva NI, Mapook A,
Jayawardena RS, Dissanayake AJ, Manawasinghe IS, Chethana
KWT, Luo ZL, Hapuarachchi KK, Baghela A, Soares AM,
Vizzini A, Meiras-Ottoni A, Mešić A, Dutta AK, de Souza CAF,
Richter C, Lin CG, Chakrabarty D, Daranagama DA, Lima DX,
Chakraborty D, Ercole E, Wu F, Simonini G, Vasquez G, da
Silva GA, Plautz Jr. HL, Ariyawansa HA, Lee H, Kušan I, Song
J, Sun J, Karmakar J, Hu K, Semwal KC, Thambugala KM,
Voigt K, Acharya K, Rajeshkumar KC, Ryvarden L, Jadan M,
Hosen MI, Mikšı́k M, Samarakoon MC, Wijayawardene NN,
Kim NM, Matočec N, Singh PN, Tian Q, Bhatt RP, de Oliveira
RJV, Tulloss RE, Aamir S, Kaewchai S, Marathe SD, Khan S,
Hongsanan S, Adhikari S, Mehmood T, Bandyopadhyay TK,
Svetasheva TY, Nguyen TTT, Antonı́n V, Li WJ, Wang Y,
Indoliya Y, Tkalčec Z, Elgorban AM, Bahkali AH, Tang AMC,
Su HY, Zhang H, Promputtha I, Luangsa-ard J, Xu J, Yan JY, JiChuan Y, Stadler M, Mortimer PE, Chomnunti P, Zhao Q,
Phillips AJL, Nontachaiyapoom S, Wen TC, Karunarathna SC
(2017) Fungal diversity notes 491–602: taxonomic and phylogenetic contributions to fungal taxa. Fungal Divers 83:1–261
Tiffany LH, Gilman JC (1965) Iowa Ascomycetes IV. Diatrypaceae.
Iowa State Coll J Sci 40:121–161
Torrejón M (2013) Fungi of Cyprus: new data on micro-and
macrofungi. Acta Mycol 48:207–218
Trakunyingcharoen T, Lombard L, Groenewald JZ, Cheewangkoon
R, Toanun C, Alfenas AC, Crous PW (2014) Mycoparasitic
species of Sphaerellopsis, and allied lichenicolous and other
genera. IMA Fungus 5:391–414
Trakunyingcharoen T, Lombard L, Groenewald JZ, Cheewangkoon
R, To-anun C, Crous PW (2015) Caulicolous Botryosphaeriales
from Thailand. Persoonia 34:87–99
Travadon R, Baumgartner K (2015) Molecular polymorphism and
phenotypic diversity in the eutypa dieback pathogen Eutypa lata.
Phytopathology 105:255–264
Travadon R, Lawrence PD, Rooney-Latham S, Gubler WD, Wilcox
WF, Rolshausen PE, Baumgartner K (2015) Cadophora species
associated with wood-decay of grapevine in North America.
Fungal Biol 119:53–66
Trouillas F, Gubler WD (2004) Identification and characterization of
Eutypa leptoplaca, a new pathogen of grapevine in Northern
California. Mycol Res 108:1195–1204
Trouillas FP, Gubler WD (2010) Pathogenicity of Diatrypaceae
species in grapevines in California. Plant Dis 94:867–872
Trouillas FP, Úrbez-Torres JR, Gubler WD (2010) Diversity of
diatrypaceous fungi associated with grapevine canker diseases in
California. Mycologia 102:319–336
Trouillas FP, Pitt WM, Sosnowski MR, Huang R, Peduto F,
Loschiavo A, Savocchia S, Scott ES (2011) Taxonomy and
DNA phylogeny of Diatrypaceae associated with Vitis vinifera
and other woody plants in Australia. Fungal Divers 49:203–223
Tsui CKM, Hyde KD, Hodgkiss IJ (2001) Colonization patterns of
wood-inhabiting fungi on baits in Hong Kong rivers, with
reference to the effects of organic pollution. Antonie Van
Leeuwenhoek J Microb 79:33–38
Tubaki K (1958) Studies on the Japanese Hyphomycetes. V J Hattori
Bot Lab 20:142–244
Udayanga D, Liu X, McKenzie EHC, Chukeatirote E, Bahkali AHA,
Hyde KD (2011) The genus Phomopsis: biology, applications,
species concepts and names of common phytopathogens. Fungal
Divers 50:189–225
123
Fungal Diversity (2018) 90:1–84
Udayanga D, Liu X-Z, Crous PW, McKenzie EHC, Chukeatirote E,
Hyde KD (2012) A multi-locus phylogenetic evaluation of
Diaporthe (Phomopsis). Fungal Divers 56:157–171
Udayanga D, Castlebury LA, Rossman AY, Chukeatirote E, Hyde KD
(2014a) Insights into the genus Diaporthe: phylogenetic species
delimitation in the D. eres species complex. Fungal Divers
67:203–229
Udayanga D, Castlebury LA, Rossman AY, Hyde KD (2014b)
Species limits in Diaporthe: molecular re-assessment of D. citri,
D. cytosporella, D. foeniculina and D. rudis. Persoonia
32:83–101
Uecker FA, Kuo K-C (1992) A new Phomopsis with long paraphyses.
Mycotaxon 44:425–433
Unamuno PLM (1941) Enumeracion y distribucion geografica de los
ascomicetos de la Peninsula Iberica y de las Islas Baleares. Mem
Real Acad Ci Exact Madrid 8:1–403
Underhill DM, Iliev ID (2014) The mycobiota: interactions between
commensal fungi and the host immune system. Nat Rev
Immunol 14:405–416
Úrbez-Torres JR (2011) The status of Botryosphaeriaceae species
infecting grapevines. Phytopathol Mediterr 50:5–45
Úrbez-Torres JR, Gubler WD (2009) Pathogenicity of Botryosphaeriaceae species isolated from grapevine cankers in California.
Plant Dis 93:584–592
Úrbez-Torres JR, Leavitt GM, Voegel TM, Gubler WD (2006)
Identification and distribution of Botryosphaeria spp. associated
with grapevine cankers in California. Plant Dis 90:1490–1503
Úrbez-Torres JR, Gubler WD, Luque J (2007) First report of
Botryosphaeria iberica and B. viticola associated with grapevine
decline in California. Plant Dis 91:772
Úrbez-Torres JR, Battany M, Bettiga LJ, Gispert C, McGourty G,
Roncoroni J, Smith RJ, Verdegaal P, Gubler WD (2010a)
Botryosphaeriaceae species spore-trapping studies in California
vineyards. Plant Dis 94:717–724
Úrbez-Torres JR, Peduto F, Gubler WD (2010b) First report of
grapevine cankers caused by Lasiodiplodia crassispora and
Neofusicoccum mediterraneum in California. Plant Dis 94:785
Úrbez-Torres JR, Peduto F, Rooney-Latham S, Gubler WD (2010c)
First report of Diplodia corticola causing grapevine (Vitis
vinifera) cankers and trunk cankers and dieback of canyon live
oak (Quercus chrysolepis) in California. Plant Dis 94:785
Úrbez-Torres JR, Peduto F, Striegler RK, Urrea-Romero KE, Rupe
JC, Cartwright RD, Gubler WD (2012) Characterization of
fungal pathogens associated with grapevine trunk diseases in
Arkansas and Missouri. Fungal Divers 52:169–189
Úrbez-Torres JR, Peduto F, Vossen PM, Krueger WH, Gubler WD
(2013a) Olive twig and branch dieback: etiology, incidence, and
distribution in California. Plant Dis 97:231–244
Úrbez-Torres JR, Peduto F, Smith RJ, Gubler WD (2013b) Phomopsis
dieback: a grapevine trunk disease caused by Phomopsis viticola
in California. Plant Dis 97:1571–1579
Úrbez-Torres JR, Haag P, Bowen P, O’Gorman DT (2014) Grapevine
trunk diseases in British Columbia: incidence and characterization of the fungal pathogens associated with black foot disease of
Grapevine. Plant Dis 98:456–468
Úrbez-Torres JR, Adams P, Kamas J, Gubler WD (2009) Identification, incidence, and pathogenicity of fungal species associated
with grapevine dieback in Texas. Am J Enol Vitic 60:497–507
Urquhart EJ, Sun LJ, Punja ZK (1997) Identification of species of
Tilletiopsis using random amplified polymorphic DNA analysis.
Can J Plant Pathol 19:380–389
Urtiaga R (1986) Indice de enfermedades en plantas de Venezuela y
Cuba. Impresos en Impresos Nuevo Siglo. S.R.L., Barquisimeto,
Venezuela
Fungal Diversity (2018) 90:1–84
Uzuhashi S, Tojo M, Kakishima M (2010) Phylogeny of the genus
Pythium and description of new genera. Mycoscience
51:337–365
Váczy KZ (2017) First report of Seimatosporium vitis associated with
grapevine trunk disease symptoms in Hungary. Plant Dis
101:253
Vail ME, Gubler WD, Adaskaveg JE (1995) First report of Pleurotus
ostreatus causing a wood rot of grapevines in California
vineyards. Plant Dis 79:1187
Valencia D, Torres C, Camps R, López E, Celis-Diez JL, Besoain X
(2015) Dissemination of Botryosphaeriaceae conidia in vineyards in the semiarid Mediterranean climate of the Valparaı́so
Region of Chile. Phytopathol Mediterr 54:394
Van Coller GJ, Denman S, Groenewald JZ, Lamprecht SC, Crous PW
(2005) Characterisation and pathogenicity of Cylindrocladiella
spp. associated with root and cutting rot symptoms of grapevines
in nurseries. Australas Plant Pathol 34:489–498
Van Niekerk JM, Crous PW, Groenewald JZ, Fourie PH, Halleen F
(2004a) DNA phylogeny, morphology and pathogenicity of
Botryosphaeria species on grapevines. Mycologia 96:781–798
Van Niekerk JM, Groenewald JZ, Verkley GJM, Fourie PH, Wingfeld
MJ, Crous PW (2004b) Systematic reappraisal of Coniella and
Pilidiella, with specific reference to species ocurring on
Eucalyptus and Vitis in South Africa. Mycol Res 108:283–303
Van Niekerk JM, Groenewald JZ, Farr DF, Fourie PH, Halleen F,
Crous PW (2005) Reassessment of Phomopsis species on
grapevines. Australas Plant Pathol 34:27–39
Van Niekerk JM, Fourie PH, Halleen F, Crous PW (2006) Botryosphaeria spp. as grapevine trunk disease pathogens. Phytopathol
Mediterr 45:S43–S54
Van Niekerk JM, Bester W, Halleen F, Crous PW, Fourie PH (2010)
First report of Lasiodiplodia crassispora as a pathogen of
grapevine trunks in South Africa. Plant Dis 94:1063
Vandenkoornhuyse P, Quaiser A, Duhamel M, Le Van A, Dufresne A
(2015) The importance of the microbiome of the plant holobiont.
New Phytol 206:1196–1206
Vanev SG, Sameva EF, Bakalova GG (1997) Order Sphaeropsidales.
Fungi Bulga 3:1–335
Vasilyeva LN (1990) New pyrenomycetous species from Kunashir.
Mikol Fitopatol 24:207–210
Vasilyeva L, Li Y, Stephenson S (2009) Some pyrenomycetous fungi
new to China. Mycotaxon 109:415–428
Vasilyeva L, Chernyshev A, Stephenson SL (2010) Pyrenomycetes of
the Russian Far East 4: Family Nitschkiaceae (Coronophorales,
Ascomycota). Mycologia 102:233–247
Vasudeva RS (1963) Indian Cercosporae. Indian Council of Agricultural Research, New Delhi
Verkley GJM, Dukik K, Renfurm R, Goker M, Stielow JB (2014)
Novel genera and species of coniothyrium-like fungi in
Montagnulaceae (Ascomycota). Persoonia 32:25–51
Victor D, Crous PW, Janse BJH, Van Zyl WH, Wingfield MJ, Alfenas
AC (1998) Systematic appraisal of species complexes within
Cylindrocladiella. Mycol Res 102:273–279
Vitale A, Castello I, Polizzi G (2008) First report of Aspergillus vine
canker on table grapes caused by Aspergillus niger in Europe.
Plant Dis 92:1471
Voglmayr H, Riethmuller A, Goker M, Weiss MJ, Oberwinkler F
(2004) Phylogenetic relationships of Plasmopara, Bremia and
other genera of downy mildew pathogens with pyriform
haustoria based on Bayesian analysis of partial LSU rDNA
sequence data. Mycol Res 108:1011–1024
Vohnı́k M, Burdı́ková Z, Vyhnal A, Koukol O (2011) Interactions
between testate amoebae and saprotrophic microfungi in a Scots
pine litter microcosm. Microb Ecol 61:660–668
von Arx JA, Mueller E (1954) Die Gattungen der amerosporen
Pyrenomyceten. Beitr Kryptogamenfl Schweiz 11:1–434
83
Voytyuk SO, Heluta VP, Wasser SP, Nevo E, Takamatsu S, Volz PA
(2009) Biodiversity of the Powdery Mildew Fungi (Erysiphales,
Ascomycota) of Israel: biodiversity of cyanoprocaryotes, algae
and fungi of Israel, vol 7. Koeltz Scientific Books, Königstein
Walker A-S, Gautier A, Confais J, Martinho D, Viaud M, Le Pecheur
P, Dupont J, Fournier E (2011) Botrytis pseudocinerea, a new
cryptic species causing gray mold in French vineyards in
sympatry with Botrytis cinerea. Phytopathology 101:1433–1445
Wang HK, Hyde KD, Soytong K, Lin FC (2008) Fungal diversity on
fallen leaves of Ficus in northern Thailand. J Zhejiang Univ Sci
B 9:835–841
Wang Y, Wang CW, Gao L (2015) First report of Fusarium
proliferatum causing fruit rot on grape (Vitis vinifera) in China.
Plant Dis 99:1180
Wangikar PD, Raut JG, Gopalkrishna N (1969) Drying of grape vines
caused by Hendersonula toruloidea. Indian Phytopathol
22:403–404
Ward DM, Weller R, Bateson MM (1990) 16S rRNA sequences
reveal numerous uncultured microorganisms in a natural community. Nature 345:63–65
Watson AJ (1971) Foreign bacterial and fungus diseases of food,
forage, and fiber crops. U.S.D.A. Agricultural Research Service,
Washington DC
Weber RW, Stenger E, Meffert A, Matthias HAHN (2004) Brefeldin
A production by Phoma medicaginis in dead pre-colonized plant
tissue: a strategy for habitat conquest? Mycol Res 108:662–671
Weir BS, Johnston PR, Damm U (2012) The Colletotrichum
gloeosporioides species complex. Stud Mycol 73:115–180
White TJ, Bruns T, Lee S, Taylor JW (1990) Amplification and direct
sequencing of fungal ribosomal RNA genes for phylogenetics.
In: Innis MA, Gelfand DH, Sninsky JJ, White TJ (eds) PCR
protocols: a guide to methods and applications. Academic, New
York, pp 315–322
White C-L, Halleen F, Fischer M, Mostert L (2011) Characterisation
of the fungi associated with esca diseased grapevines in South
Africa. Phytopathol Mediterr 50:204–223
Whitelaw-Weckert MA, Nair NG, Lamont R, Alonso M, Priest MJ,
Huang R (2007) Root infection of Vitis vinifera by Cylindrocarpon liriodendra in Australia. Australas Plant Pathol
36:403–406
Whitelaw-Weckert MA, Rahman L, Appleby LM, Hall A, Clark AC,
Waite H, Hardie WJ (2013) Co-infection by Botryosphaeriaceae
and Ilyonectria spp. fungi during propagation causes decline of
young grafted grapevines. Pl Pathol 62:1226–1237
Whiteside JO (1966) A revised list of plant diseases in Rhodesia.
Kirkia 5:87–196
Whiting E, Cunha MG, Gubler WD (2005) Phaeomoniella chlamydospora and Phaeoacremonium species distinguished through
cultural characters and ribosomal DNA sequence analysis.
Mycotaxon 92:351–360
Wicht B, Petrini O, Jermini M, Gessler C, Broggini GAL (2012)
Molecular, proteomic and morphological characterization of the
ascomycete Guignardia bidwellii, agent of grape black rot: a
polyphasic approach to fungal identification. Mycologia
104:1036–1045
Wiehe PO (1948) The plant diseases and fungi recorded from
Mauritius. Mycol Pap 24:1–39
Wijayawardene NN, Hyde KD, Rajeshkumar KC, Hawksworth DL,
Madrid H, Kirk PM, Braun U, Singh RV, Crous PW, Kukwa M,
Lücking R, Kurtzman CP, Yurkov A, Haelewaters D, Aptroot A,
Lumbsch HT, Timdal E, Ertz D, Etayo J, Phillips AJL,
Groenewald JZ, Papizadeh M, Selbmann L, Dayarathne MC,
Weerakoon G, Jones EBG, Suetrong S, Tian Q, Castañeda-Ruiz
RF, Bahkali AH, Pang K-L, Tanaka K, Dai DQ, Sakayaroj J,
Hujslová M, Lombard L, Shenoy BD, Suija A,
Maharachchikumbura SSN, Thambugala KM, Wanasinghe DN,
123
84
Fungal Diversity (2018) 90:1–84
Sharma BO, Gaikwad S, Pandit G, Zucconi L, Onofri S, Egidi E,
Raja HA, Kodsueb R, Cáceres MES, Pérez-Ortega S, Fiuza PO,
Monteiro JS, Vasilyeva LN, Shivas RG, Prieto M, Wedin M,
Olariaga I, Lateef AA, Agrawal Y, Fazeli SAS, Amoozegar MA,
Zhao GZ, Pfliegler WP, Sharma G, Oset M, Abdel-Wahab MA,
Takamatsu S, Bensch K, de Silva NI, De Kesel A, Karunarathna
A, Boonmee S, Pfister DH, Lu Y-Z, Luo Z-L, Boonyuen N,
Daranagama DA, Senanayake IC, Jayasiri SC, Samarakoon MC,
Zeng X-Y, Doilom M, Quijada L, Rampadarath S, Heredia G,
Dissanayake AJ, Jayawardena RS, Perera RH, Tang L-Z,
Phukhamsakda C, Hernández-Restrepo M, Ma X, Tibpromma
S, Gusmao LFP, Weerahewa D, Karunarathna SC (2017) Notes
for genera: Ascomycota. Fungal Divers 86:1–594
Wijayawardene NN, Hyde KD, Divakar PK, Rajeshkumar KC,
Weerahewa D, Delgado G, Wang Y, Fu L (2018) Notes for
genera
update—Ascomycota:
6616–6821.
Mycosphere
9:115–140
Witbooi WR, Taylor MA, Fourie JF (2000) In vitro studies on the
effect of harvest maturity, relative humidity, wetness period and
cold-storage temperature, on the infection potential of Aspergillus niger and Rhizopus stolonifer on Thompson Seedless
table grapes. Decid Fruit Grower 50:S1–S14
Wolf FA, Garren KH, Miller JK (1938) Fungi of the Duke Forest and
their relation to forest pathology. Bull School For Duke Univ
2:1–122
Wong MKM, Hyde KD (2001) Diversity of fungi on six species of
Gramineae and one species of Cyperaceae in Hong Kong. Mycol
Res 105:1485–1491
Wu DD, Fu G, Hu FY, Ye YF, Mou HF, Qin LL, Jiang N (2015) First
report of Neofusicoccum parvum causing panicle blight and leaf
spot on Vitis heyneana in China. Plant Dis 99:417
Yan J-Y, Peng Y-L, Xie Y, Li X-H, Yao S-W, Tang M-L, Wang Z-Y
(2011a) First report of grapevine trunk disease caused by
Botryosphaeria obtusa in China. Plant Dis 95:616
Yan J-Y, Li X-H, Kong FF, Wang Z-Y, Gong L-Z, He H-P (2011b)
Occurrence of grapevine trunk disease caused by Botryosphaeria
rhodina in China. Plant Dis 95:219
Yan J, Xie Y, Yao S-W, Wang Z, Li X (2012) Characterization of
Botryosphaeria dothidea, the casual agent of grapevine canker in
China. Australas Plant Pathol 41:351–357
Yan J-Y, Jayawardena MMRS, Goonasekara ID, Wang Y, Zhang W,
Liu M, Huang J-B, Wang Z-Y, Shang J-J, Peng Y-L, Bahkali A,
Hyde KD, Li X-H (2015) Diverse species of Colletotrichum
associated with grapevine anthracnose in China. Fungal Divers
71:233–246
Yang T, Groenewald JZ, Cheewangkoon R, Jami F, Abdollahzadeh J,
Lombard L, Crous PW (2017) Families, genera, and species of
Botryosphaeriales. Fungal Biol 121:322–346
Yanna Ho WHH, Hyde KD (2002) Fungal succession on fronds of
Phoenix hanceana in Hong Kong. Fungal Divers 10:185–211
Yilmaz N, Visagie CM, Houbraken J, Frisvad JC, Samson RA (2014)
Polyphasic taxonomy of the genus Talaromyces. Stud in Mycol
78:175–341
Ying-Ren L (2012) Flora Fungorum Sinicorum: Rhytismatales, vol
40. Science Press, Beijing
Zapparata A, Da Lio D, Sarrocco S, Vannacci G, Baroncelli R (2017)
First report of Colletotrichum godetiae causing grape (Vitis
vinifera) berry rot in Italy. Plant Dis 101:1051–1052
Zervakis G, Dimou D, Balis C (1998) A check-list of the Greek
macrofungi including hosts and biogeographic distribution: I.
Basidiomycotina. Mycotaxon 66:273–336
Zhang TY (2003) Flora Fungorum Sinicorum. Alternaria, vol 16.
Science Press, Beijing
Zhang L, Zhang GL, Qian X, Li GY (2009) First report of verticillium
wilt of grapevine (Vitis vinifera) caused by Verticillium dahlia in
China. Plant Dis 93:841
Zheng RY, Liu XY (2005) Actinomucor elegans var. meitauzae, the
correct name for A. taiwanensis and Mucor meitauzae (Mucorales, Zygomycota). Nova Hedwig 80:419–432
Zhou YJ, Zhang J, Wang XD, Yang L, Jiang DH, Li GQ, Hsiang T,
Zhuang WY (2014) Morphological and phylogenetic identification of Botrytis sinoviticola, a novel cryptic species causing gray
mold disease of table grapes (Vitis vinifera) in China. Mycologia
106:43–56
Zhou N, Chen Q, Carroll G, Zhang N, Shivas RG,Cai L (2015)
Polyphasic characterization of four new plant pathogenic
Phyllosticta species from China, Japan, and the United States.
Fung Biol 119:433–446
Zhuang W-Y (ed) (2001) Higher fungi of Tropical China. Mycotaxon
Ltd, Ithaca
Zhuang W-Y (ed) (2005) Fungi of northwestern China. Mycotaxon
Ltd, Ithaca
Živkovi_c S, Vasi_c T, And̄elković S, Jevremovi_c D, Trkulja V (2012)
Identification and characterization of Eutypa lata on grapevine in
Serbia. Plant Dis 96:913–913
Zubkova RD (1971) Genus novum Saccharomycetacearum e
Kazachstania. Botanicheskie Materialy Gerbariga Instituta
Botaniki Akademii Nauk Kazakh. SSR 7:53–56
Affiliations
Ruvishika S. Jayawardena1,2,3 • Witoon Purahong4 • Wei Zhang1,3 • Tesfaye Wubet4,5 • XingHong Li1,3
Mei Liu1,3 • Wensheng Zhao6 • Kevin D. Hyde2 • JianHua Liu1 • Jiye Yan1,3
•
1
Institute of Plant and Environment Protection, Beijing
Academy of Agriculture and Forestry Sciences,
Beijing 100097, People’s Republic of China
4
Department of Soil Ecology, UFZ-Helmholtz Centre for
Environmental Research, Theodor-Lieser-Str. 4,
06120 Halle (Saale), Germany
2
Centre of Excellence in Fungal Research, Mae Fah Luang
University, Chiang Rai 57100, Thailand
5
German Centre for Integrative Biodiversity Research (iDiv)
Halle-Jena-Leipzig, Leipzig, Germany
3
Beijing Key Laboratory of Environment Friendly
Management on Fruit Diseases and Pests in North China,
Beijing 100097, People’s Republic of China
6
College of Agricultural and Biotechnology, China
Agricultural University, Beijing 100193, People’s Republic
of China
123