RESUMEN
Novel species of fungi described in this study include those from various countries as follows: Argentina, Neocamarosporium halophilum in leaf spots of Atriplex undulata. Australia, Aschersonia merianiae on scale insect (Coccoidea), Curvularia huamulaniae isolated from air, Hevansia mainiae on dead spider, Ophiocordyceps poecilometigena on Poecilometis sp. Bolivia, Lecanora menthoides on sandstone, in open semi-desert montane areas, Sticta monlueckiorum corticolous in a forest, Trichonectria epimegalosporae on apothecia of corticolous Megalospora sulphurata var. sulphurata, Trichonectria puncteliae on the thallus of Punctelia borreri. Brazil, Catenomargarita pseudocercosporicola (incl. Catenomargarita gen. nov.) hyperparasitic on Pseudocercospora fijiensis on leaves of Musa acuminata, Tulasnella restingae on protocorms and roots of Epidendrum fulgens. Bulgaria, Anthracoidea umbrosae on Carex spp. Croatia, Hymenoscyphus radicis from surface-sterilised, asymptomatic roots of Microthlaspi erraticum, Orbilia multiserpentina on wood of decorticated branches of Quercus pubescens. France, Calosporella punctatispora on dead corticated twigs of Aceropalus. French West Indies (Martinique), Eutypella lechatii on dead corticated palm stem. Germany, Arrhenia alcalinophila on loamy soil. Iceland, Cistella blauvikensis on dead grass (Poaceae). India, Fulvifomes maritimus on living Peltophorum pterocarpum, Fulvifomes natarajanii on dead wood of Prosopis juliflora, Fulvifomes subazonatus on trunk of Azadirachta indica, Macrolepiota bharadwajii on moist soil near the forest, Narcissea delicata on decaying elephant dung, Paramyrothecium indicum on living leaves of Hibiscus hispidissimus, Trichoglossum syamviswanathii on moist soil near the base of a bamboo plantation. Iran, Vacuiphoma astragalicola from stem canker of Astragalus sarcocolla. Malaysia, Neoeriomycopsis fissistigmae (incl. Neoeriomycopsidaceae fam. nov.) on leaf spots on flower Fissistigma sp. Namibia, Exophiala lichenicola lichenicolous on Acarospora cf. luederitzensis. Netherlands, Entoloma occultatum on soil, Extremus caricis on dead leaves of Carex sp., Inocybe pseudomytiliodora on loamy soil. Norway, Inocybe guldeniae on calcareous soil, Inocybe rupestroides on gravelly soil. Pakistan, Hymenagaricus brunneodiscus on soil. Philippines, Ophiocordyceps philippinensis parasitic on Asilus sp. Poland, Hawksworthiomyces ciconiae isolated from Ciconia ciconia nest, Plectosphaerella vigrensis from leaf spots on Impatiens noli-tangere, Xenoramularia epitaxicola from sooty mould community on Taxus baccata. Portugal, Inocybe dagamae on clay soil. Saudi Arabia, Diaporthe jazanensis on branches of Coffea arabica. South Africa, Alternaria moraeae on dead leaves of Moraea sp., Bonitomyces buffels-kloofinus (incl. Bonitomyces gen. nov.) on dead twigs of unknown tree, Constrictochalara koukolii on living leaves of Itea rhamnoides colonised by a Meliola sp., Cylindromonium lichenophilum on Parmelina tiliacea, Gamszarella buffelskloofina (incl. Gamszarella gen. nov.) on dead insect, Isthmosporiella africana (incl. Isthmosporiella gen. nov.) on dead twigs of unknown tree, Nothoeucasphaeria buffelskloofina (incl. Nothoeucasphaeria gen. nov.), on dead twigs of unknown tree, Nothomicrothyrium beaucarneae (incl. Nothomicrothyrium gen. nov.) on dead leaves of Beaucarnea stricta, Paramycosphaerella proteae on living leaves of Protea caffra, Querciphoma foliicola on leaf litter, Rachicladosporium conostomii on dead twigs of Conostomium natalense var. glabrum, Rhamphoriopsis synnematosa on dead twig of unknown tree, Waltergamsia mpumalanga on dead leaves of unknown tree. Spain, Amanita fulvogrisea on limestone soil, in mixed forest, Amanita herculis in open Quercus forest, Vuilleminia beltraniae on Cistus symphytifolius. Sweden, Pachyella pulchella on decaying wood on sand-silt riverbank. Thailand, Deniquelata cassiae on dead stem of Cassia fistula, Stomiopeltis thailandica on dead twigs of Magnolia champaca. Ukraine, Circinaria podoliana on natural limestone outcrops, Neonematogonum carpinicola (incl. Neonematogonum gen. nov.) on dead branches of Carpinus betulus. USA, Exophiala wilsonii water from cooling tower, Hygrophorus aesculeticola on soil in mixed forest, and Neocelosporium aereum from air in a house attic. Morphological and culture characteristics are supported by DNA barcodes. Citation: Crous PW, Costa MM, Kandemir H, et al. 2023. Fungal Planet description sheets: 1550-1613. Persoonia 51: 280-417. doi: 10.3767/persoonia.2023.51.08.
RESUMEN
Kura clover (Trifolium ambiguum M. Bieb.), a rhizomatous, persistent legume native to the Caucasus region, has received recent attention in North America and New Zealand as a pasture and silage crop. It is reported to be resistant to most pathogens affecting other clovers, including Sclerotinia trifoliorum Eriks. (3,4), one of the most destructive pathogens of clovers in northern Europe. Kura clover (cv. KTA202) was established in May 2009 near Mochelek, Poland (53° 13' N, 17° 51' E) on a Luvisol soil. By May 2011, 70% of plants grown in an experimental field (350 m2) had died, and 20% of the remaining plants were yellow and wilted. At crowns and the lower stem regions, wet, brown lesions with delicate white mycelium were observed. Lesion development was followed by death of the entire plant in a few days. By early June, only a few asymptomatic plants per square meter remained in the field. Tissue fragments of 20 symptomatic plants were surface-sterilized with 1% NaOCl for 1 min and plated on potato dextrose agar (PDA). A fungus with morphological characteristics of S. trifoliorum was consistently isolated. DNA isolation from sclerotia was performed with the DNeasy Plant Mini Kit (Qiagen, USA). Amplification and sequencing of the ITS region of rDNA was performed with primers ITS1/ITS4. NCBI Blast analysis of the 542-bp segment showed a 99% homology with most of S. trifoliorum and S. sclerotiorum strains in GenBank (e.g., AY547267.1 and EU082466.1). Sequence of isolate St0211TA was deposited in GenBank (Accession No. JQ743329). To determine growth rate of hyphae, morphology, and dimensions of sclerotia, colonies were grown in three replications on PDA at 20 ± 1°C in the dark. S. trifoliorum (CBS 122377) and S. sclerotiorum from our local collection were used as controls. Mean growth rate of S. trifoliorum isolates (20.5 mm/day) was slower compared to S. sclerotiorum (32.3 mm/day). Sclerotia began to form on delicate and smooth mycelium of S. trifoliorum on the entire surface of the plate in 7 to 8 days. Sclerotial size on day 28 was 2.0 to 9.0 × 2.0 to 7.0 mm (average 4.2 × 3.6 mm). Ultimately, the identification of S. trifoliorum was confirmed on the basis of ascospore morphology. Apothecia grew from sclerotia in wet sand at 12°C after 12 weeks. Asci contained dimorphic ascospores: four larger 13.0 to 16.0 × 6.0 to 9.0 mm (average 14.1 × 7.4 µm) and four smaller 10.0 to 12.0 × 5.4 to 6.0 mm (average 10.6 × 6.0 µm), typical for this species (1). Isolate St0511TA, which most intensively produced apothecia, was deposited in CBS (No. 133234). Koch's postulates were fulfilled by pathogenicity tests carried out on 2-week-old T. ambiguum seedlings grown in pots (6 × 30 plants), sprayed with a mycelial fragment suspension, and incubated at 15°C (2). Brown, wet spots with delicate white mycelium were observed on cotyledons after 3 days. After 5 days, approximately 10% of cotyledons were killed and mycelium appeared on stems and leaves, and after 10 days, 73% of seedlings were dead. S. trifoliorum was reisolated from all symptomatic tissues. To our knowledge, this is the first report of S. trifoliorum stem blight on T. ambiguum in the field. References: (1) E. N. Njambere et al. Plant Dis. 92:917, 2008. (2) L. H. Rhodes, Sclerotinia Crown and Stem Rot Resistance, http://www.naaic.org/stdtests/scleroti.htm , 1991. (3) A. K. Slesaravichyus et al., Selektsiya i Semenovodstvo Moskva 6:21, 1988. (4) N. L. Taylor and R. R. Smith, Adv. Agron. 63:153, 1998.
