New Cladosporium Species from Normal and Galled Flowers of Lamiaceae.

A series of isolates of Cladosporium spp. were recovered in the course of a cooperative study on galls formed by midges of the genus Asphondylia (Diptera, Cecidomyidae) on several species of Lamiaceae. The finding of these fungi in both normal and galled flowers was taken as an indication that they do not have a definite relationship with the midges. Moreover, identification based on DNA sequencing showed that these isolates are taxonomically heterogeneous and belong to several species which are classified in two different species complexes. Two new species, Cladosporium polonicum and Cladosporium neapolitanum, were characterized within the Cladosporium cladosporioides species complex based on strains from Poland and Italy, respectively. Evidence concerning the possible existence of additional taxa within the collective species C. cladosporioides and C. pseudocladosporioides is discussed.

1. Introduction

Fungi belonging to the genus Cladosporium (Dothideomycetes, Cladosporiaceae) are ubiquitous and reported to be able to colonize a huge diversity of substrates in any natural or anthropized environment on earth [1]. They are well known as plant disease agents [1,2,3,4,5], but also reported as pathogens of animals [6] and humans [7,8,9], and are considered among the most widespread fungi in buildings and indoor environments [10]. Other species are endophytic or have been reported from soil, dung or leaf litter [11,12,13,14]. Recent investigations have shown that pathogenic strains usually belong to species mostly known as saprophytes, underlining the importance of an accurate assessment of the phylogenetic relationships for the identification of specialized lineages and possible cryptic species [1,7,8,10]. In fact, classification based on morphology has proved to be problematic due to the infrequency of the perfect stage and the absence of outstanding differences in the conidial structures, so that culturing and microscope observations only allowed a partial separation of taxa possibly representing collective species. Therefore, widespread species, such as C. cladosporioides, C. herbarum, and C. sphaerospermum, are now regarded as species complexes (s.c.), disclosing a broader variation as and when the characterization of new strains proceeds from new ecological contexts and geographic areas [3]. Indeed, the easier access to DNA sequencing and online databases is ongoingly supporting the distinction of novel species, to such an extent that within the C. cladosporioides s.c. their number has currently raised up to 67 (Table 1).

Table 1

List of Cladosporium strains from accepted taxa and their corresponding DNA sequences which have been used in the phylogenetic analyses.

Species	Code	Host	Country	ITS	TEF1	ACT
C. acalyphae	CBS 125982	Acalypha australis	South Korea	HM147994	HM148235	HM148481
C. alboflavescens	CBS 140690	bronchoalveolar lavage fluid	United States	LN834420	LN834516	LN834604
C. angulosum	CPC 22271	indoor air	United States	MF472918	MF473345	MF473768
C. angulosum	CBS 140692	bronchoalveolar lavage fluid	United States	LN834425	LN834521	LN834609
C. angustisporum	CBS 125983	Alloxylon wickhamii	Australia	HM147995	HM148236	HM148482
C. angustisporum	DTO-127-E6	air in bakery	United States	KP701935	KP701812	KP702057
C. angustiterminale	CBS 140480	Banksia grandis	Australia	KT600379	KT600476	KT600575
C. anthropophilum	CBS 117483	-	United States	HM148007	HM148248	HM148494
C. anthropophilum	CPC 22393	indoor air	United States	MF472922	MF473349	MF473772
C. arenosum	CHFC-EA 566	marine sediment	Antarctica	MN879328	MN890011	MN890008
C. asperulatum	CBS 126340	Protea susannae	Portugal	HM147998	HM148239	HM148485
C. asperulatum	CBS 126339	leaf litter	India	HM147997	HM148238	HM148484
C. australiense	DTO-255-F3	bathroom	Netherlands	KP701978	KP701855	KP702100
C. australiense	CBS 125984	Eucalyptus moluccana	Australia	HM147999	HM148240	HM148486
C. austroafricanum	CBS 140481	leaf litter	South Africa	KT600381	KT600478	KT600577
C. chalastosporoides	CBS 125985	Teratosphaeria proteae-arboreae on Protea arborea	South Africa	HM148001	HM148242	HM148488
C. chasmanthicola	CBS 142612	Chasmanthe aethiopica	South Africa	KY646221	KY646227	KY646224
C. chubutense	CBS 124457	Pinus ponderosa	Argentina	FJ936158	FJ936161	FJ936165
C. cladosporioides	CBS 113739	crested wheat grass	United States	HM148005	HM148246	HM148492
C. cladosporioides	CBS 145.35	Pisum sativum	Germany	HM148013	HM148254	HM148500
C. cladosporioides	CBS 101367	soil	Brazil	HM148002	HM148243	HM148489
C. cladosporioides	CBS 112388	indoor air	Germany	HM148003	HM148244	HM148490
C. cladosporioides	CPC 15615	wild tree	Mexico	KT600386	KT600483	KT600581
C. cladosporioides	CPC 22367	indoor air	United States	MF472941	MF473368	MF473791
C. cladosporioides	CPC 14271	unidentified tree	France	HM148045	HM148286	HM148532
C. cladosporioides	CPC 15626	wild plant	Mexico	KT600387	KT600484	KT600582
C. colocasiae	CBS 386.64	Colocasia esculenta	Taiwan	HM148067	HM148310	HM148555
C. colocasiae	CBS 119542	Colocasia esculenta	Japan	HM148066	HM148309	HM148554
C. colombiae	CBS 274.80B	Cortaderia sp.	Colombia	FJ936159	FJ936163	FJ936166
C. crousii	CBS 140686	bronchoalveolar lavage fluid	United States	LN834431	LN834527	LN834615
C. cucumerinum	CBS 174.62	painted floor	United States	HM148076	HM148320	HM148565
C. cucumerinum	CBS 174.54	Cucumis sativus	Netherlands	HM148075	HM148319	HM148564
C. delicatulum	CBS 126342	indoor air	Denmark	HM148079	HM148323	HM148568
C. delicatulum	CBS 126344	Tilia cordata	Germany	HM148081	HM148325	HM148570
C. europaeum	CBS 134914	building material	Denmark	HM148056	HM148298	HM148543
C. europaeum	CPC 14238	fruit of Sambucus nigra	Netherlands	HM148055	HM148297	HM148542
C. exasperatum	CBS 125986	Eucalyptus tintinnans	Australia	HM148090	HM148334	HM148579
C. exile	CBS 125987	Phyllactinia guttata on leaf of Corylus sp.	United States	HM148091	HM148335	HM148580
C. flabelliforme	CBS 126345	Melaleuca cajuputi	Australia	HM148092	HM148336	HM148581
C. flavovirens	CBS 140462	toe nail	United States	LN834440	LN834536	LN834624
C. funiculosum	CBS 122129	Vigna umbellata	Japan	HM148094	HM148338	HM148583
C. funiculosum	CBS 122128	Ficus carica	Japan	HM148093	HM148337	HM148582
C. gamsianum	CBS 125989	Strelitzia sp.	South Africa	HM148095	HM148339	HM148584
C. gamsianum	CPC 15617	seeds of Glycine max	Mexico	KT600392	KT600489	KT600587
C. globisporum	CBS 812.96	meat stamp	Sweden	HM148096	HM148340	HM148585
C. globisporum	DTO-220-D4	indoor environment	Netherlands	KP701967	KP701844	KP702089
C. grevilleae	CBS 114271	leaf of Grevillea sp.	Australia	JF770450	JF770472	JF770473
C. hillianum	CBS 125988	leaf of Typha orientalis	New Zealand	HM148097	HM148341	HM148586
C. hillianum	CPC 15458	leaf of Typha orientalis	New Zealand	HM148098	HM148342	HM148587
C. inversicolor	CBS 401.80	Triticum aestivum	Netherlands	HM148101	HM148345	HM148590
C. inversicolor	DTO-108-F8	indoor environment	France	KP701908	KP701785	KP702031
C. ipereniae	CBS 140483	Puya sp.	Chile	KT600394	KT600491	KT600589
C. ipereniae	CPC 16855	Arctostaphylos pallida	United States	KT600395	KT600492	KT600590
C. iranicum	CBS 126346	leaf of Citrus sinensis	Iran	HM148110	HM148354	HM148599
C. kenpeggii	CBS 142613	leaf of Passiflora edulis	Australia	KY646222	KY646228	KY646225
C. licheniphilum	CBS 125990	Physcia sp.	Germany	HM148111	HM148355	HM148600
C. longicatenatum	CBS 140485	unknown plant	Australia	KT600403	KT600500	KT600598
C. lycoperdinum	CBS 274.80C	Puya sp.	Colombia	HM148114	HM148358	HM148603
C. lycoperdinum	CBS 126347	gall of Apiosporina morbosa on Prunus sp.	Canada	HM148112	HM148601	HM148601
C. montecillanum	CBS 140486	pine needles	Mexico	KT600406	KT600504	KT600602
C. montecillanum	CPC 15605	Taraxacum sp.	Mexico	KT600407	KT600505	KT600603
C. myrtacaearum	CBS 126350	Corymbia foelscheana	Australia	HM148117	HM148361	HM148606
C. myrtacaearum	CBS 126349	Eucalyptus placita	Australia	MH863925	HM148360	HM148605
C. needhamense	CBS 143359	indoor air sample	United States	MF473142	MF473570	MF473991
C. neerlandicum	CBS 143360	archive dust	Netherlands	KP701887	KP701764	KP702010
C. neopsychrotolerans	CGMCC3.18031	rhizosphere of Saussurea involucrata	China	KX938383	KX938400	KX938366
C. neopsychrotolerans	CGMCC3.18032	rhizosphere of Saussurea involucrata	China	KX938384	KX938401	KX938367
C. oxysporum	CBS 125991	soil	China	HM148118	HM148362	HM148607
C. oxysporum	CBS 126351	indoor air	Venezuela	HM148119	HM148363	HM148608
C. paracladosporioides	CBS 171.54	-	-	HM148120	HM148364	HM148609
C. parapenidielloides	CBS 140487	Eucalyptus sp.	Australia	KT600410	KT600508	KT600606
C. perangustum	CBS 125996	Cussonia sp.	South Africa	HM148121	HM148365	HM148610
C. perangustum	CBS 126365	Phyllactinia guttata on leaf of Corylus sp.	United States	MH863940	HM148367	HM148612
C. phaenocomae	CBS 128769	Phaenocoma prolifera	South Africa	JF499837	JF499875	JF499881
C. phaenocomae	CPC 18221	Phaenocoma prolifera	South Africa	JF499838	JF499876	JF499882
C. phyllactiniicola	CBS 126354	Phyllactinia guttata on leaf of Corylus sp.	United States	MH863930	HM148396	HM148641
C. phyllactiniicola	CBS 126355	Phyllactinia guttata on leaf of Corylus sp.	United States	HM148153	HM148397	HM148642
C. phyllophilum	CBS 125992	Taphrina sp. on Prunus cerasus	Germany	HM148154	HM148398	HM148643
C. phyllophilum	CPC 13873	Teratosphaeria proteae-arboreae on Protea arborea	South Africa	HM148155	HM148399	HM148644
C. pini-ponderosae	CBS 124456	Pinus ponderosa	Argentina	FJ936160	FJ936164	FJ936167
C. pseudochalastosporoides	CBS 140490	pine needles	Mexico	KT600415	KT600513	KT600611
C. pseudocladosporioides	CBS 125993	air	Netherlands	HM148158	HM148402	HM148647
C. pseudocladosporioides	CBS 117153	leaf of Paeonia sp.	Germany	HM148157	HM148401	HM148646
C. ramotenellum	CPC 14300	building material	Denmark	KT600438	KT600537	KT600635
C. rectoides	CBS 125994	Vitis flexuosa	South Korea	HM148193	HM148438	HM148683
C. rectoides	CBS 126357	Plectranthus sp.	South Korea	MH863933	HM148439	HM148684
C. rugulovarians	CBS 140495	unidentified Poaceae	Brazil	KT600459	KT600558	KT600656
C. scabrellum	CBS 126358	Ruscus hypoglossum	Slovenia	HM148195	HM148440	HM148685
C. silenes	CBS 109082	Silene uniflora	United Kingdom	EF679354	EF679429	EF679506
C. silenes	MFLUCC 17-0195	Vitis vinifera	China	MG938717	MG938830	MG938682
C. sinuatum	CGMCC3.18096	soil	China	KX938385	KX938402	KX938368
C. sinuatum	CGMCC3.18097	soil	China	KX938386	KX938403	KX938369
Cladosporium sp.	UTHSC DI-13-227	human sputum	United States	LN834422	LN834518	LN834606
Cladosporium sp.	UTHSC DI-13-245	toe	United States	LN834429	LN834525	LN834613
Cladosporium sp.	UTHSC DI-13-265	bronchoalveolar lavage fluid	United States	LN834435	LN834531	LN834619
Cladosporium sp.	UTHSC DI-13-218	bronchoalveolar lavage fluid	United States	LN834418	LN834514	LN834602
Cladosporium sp.	UTHSC DI-13-210	human skin	United States	LN834414	LN834510	LN834598
C. subuliforme	CBS 126500	Chamaedorea metallica	Thailand	HM148196	HM148441	HM148686
C. subuliforme	DTO-130-H8	indoor environment	Thailand	KP701938	KP701815	KP702060
C. tenuissimum	XCSY3	Coriandrum sativum	China	MG873079	MT154184	MT154174
C. tenuissimum	CBS 125995	Lagerstoemia sp.	United States	HM148197	HM148442	HM148687
C. tianshanense	CGMCC3.18033	rhizosphere of Saussurea involucrata	China	KX938381	KX938398	KX938364
C. tianshanense	CGMCC3.18034	rhizosphere of Saussurea involucrata	China	KX938382	KX938399	KX938365
C. uredinicola	CPC 5390	Cronartium fusiforme on Quercus nigra	United States	AY251071	HM148467	HM148712
C. uwebraunianum	CBS 143365	indoor air	Netherlands	MF473306	MF473729	MF474156
C. uwebraunianum	DTO-305-H9	house dust	New Zealand	MF473307	MF473730	MF474157
C. varians	CBS 126361	leaf debris	India	MH863937	HM148469	HM148714
C. varians	CBS 126362	Catalpa bungei	Russia	HM148224	HM148470	HM148715
C. verrucocladosporioides	CBS 126363	Rhus chinensis	South Korea	HM148226	HM148472	HM148717
C. vicinum	CBS 143366	indoor air	United States	MF473311	MF473734	MF474161
C. vicinum	CBS 306.84	uredospore of Puccinia allii	United Kingdom	HM148057	HM148299	HM148544
C. vignae	CBS 121.25	Vigna unguiculata	United States	HM148227	HM148473	HM148718
C. welwitschiicola	CPC 18648	Welwitschia mirabilis	Namibia	KY646223	KY646229	KY646226
C. westerdijkiae	CPC 10150	Fatoua villosa	South Korea	HM148062	HM148304	HM148549
C. westerdijkiae	CPC 14284	Triticum sp.	Germany	HM148065	HM148307	HM148552
C. xanthocromaticum	CBS 126364	Erythrophleum chlorostachys	Australia	HM148122	HM148366	HM148611
C. xanthocromaticum	CPC 22239	indoor air	United States	MF473316	MF473739	MF474166
C. xylophilum	CBS 125997	dead wood of Picea abies	Russia	HM148230	HM148476	HM148721
C. xylophilum	CBS 113749	Prunus avium	United States	HM148228	HM148474	HM148719

One of the most fruitful investigational fields on the occurrence of Cladosporium species is represented by the ecological interactions with other organisms. Particularly, many studies have evidenced the ability of these fungi to exert antagonistic effects against pests and pathogens of crops, which is also supported by their widespread association with plants as epiphytes or endophytes [15,16]. However, in other cases it has not been clearly established whether the finding of Cladosporium is related to a definite symbiotic interaction or to a merely saprophytic condition. One of these cases is represented by the association with midges belonging to the Asphondyliinae (Diptera, Cecidomyidae), which on many plant species induce the formation of galls where larvae develop by feeding on a mycelial mat lining the gall walls. The fungal counterpart was identified as Cladosporium sp. in early investigations on these peculiar symbiotic associations [17,18]. Later on, this role was questioned, although occurrence of Cladosporium in galls was confirmed in recent reports from several plants and countries worldwide [19,20,21]. Moreover, the finding of Cladosporium conidia in mycangia and on the body surface of egg-laying midges could possibly support the conjecture that the insect may actively spread the fungus during oviposition [21,22].

In the course of a cooperative investigational activity on the fungal associates developing in galls produced by midges of the genus Asphondylia in flowers of several species of Lamiaceae [23,24], strains of Cladosporium were frequently recovered during the isolation attempts. However, unlike Botryosphaeria dothidea which was only isolated from galls [25], Cladosporium isolates were also obtained from the inner parts of normal flowers and from achenes, indicating that their presence in the flower microenvironment is independent by the insect, and is likely to not affect flower physiology. In the absence of previous assessments, identification at species level appeared to be fundamental in order to conclusively establish whether these isolates are taxonomically homogeneous, hence, to be possibly regarded as specialized gall associates, or rather occur as unrelated saprophytes.

2. Results

2.1. Cladosporium Isolates

As discussed above, Cladosporium strains were quite frequently isolated from flower galls, their inquiline insects and normal flowers collected on several Lamiaceae species examined in our investigation. Forty strains from the resulting collection were selected to be examined in this study (Table 2). The list included representatives from all the sampled plant species, with a prevalence of isolates from galls depending on the higher number of isolations which were performed from this source.

Table 2

List of Cladosporium isolates recovered from galled and non-galled flowers of Lamiaceae which have been considered in the present study, with GenBank codes of the deposited DNA sequences.

Strain	Source	Location	ITS	TEF1	ACT
AjNa1	Ajuga reptans—receptacle	Napoli	MK387884	MK416088	MK416045
AcAv2	Clinopodium nepeta—achene	Averno	MK387911	MK416115	MK416072
AcAv4	Clinopodium nepeta—larva of A. nepetae	Averno	MK387888	MK416092	MK416049
AcAv16	Clinopodium nepeta—larva of parasitoid	Averno	MK387905	MK416109	MK416066
AcBa1	Clinopodium nepeta—larva of A. nepetae	Napoli	MK387916	MK416120	MK416077
AcBa2	Clinopodium nepeta—gall wall	Napoli	MK387899	MK416103	MK416060
AcBa3	Clinopodium nepeta—gall wall	Napoli	MK387917	MK416121	MK416078
AcBa8	Clinopodium nepeta—larva of parasitoid	Napoli	MK387906	MK416110	MK416067
AcCe1	Clinopodium nepeta—gall wall	Caserta	MK387910	MK416114	MK416071
AcMn6	Clinopodium nepeta—gall wall	Montenuovo	MK387914	MK416118	MK416075
AcMt5	Clinopodium nepeta—gall wall	Matera	MK387880	MK416084	MK416041
AcMt6	Clinopodium nepeta—larva of A. nepetae	Matera	MK387883	MK416087	MK416044
AcNa1	Clinopodium nepeta—gall wall	Astroni	MK387881	MK416085	MK416042
AcPp1	Clinopodium nepeta—gall wall	Pietrapertosa	MK387900	MK416104	MK416061
AcPp2	Clinopodium nepeta—receptacle	Pietrapertosa	MK387885	MK416089	MK416046
AcRi7	Clinopodium nepeta—receptacle	Rivello	MK387886	MK416090	MK416047
SG8	Clinopodium nepeta—gall wall	San Giorgio a Cremano	MK387907	MK416111	MK416068
CL1	Clinopodium vulgare—gall wall	Rivello	MK387908	MK416112	MK416069
CL3	Clinopodium vulgare—gall wall	Rivello	MK387898	MK416102	MK416059
CL4	Clinopodium vulgare—achene	Rivello	MK387904	MK416108	MK416065
S1	Clinopodium vulgare—achene	Grunau im Almtal	MK387902	MK416106	MK416063
LaPo1	Lamiastrum sp.—receptacle	Pontone	MK387878	MK416082	MK416039
LaNa1	Lamium album—receptacle	Napoli	MK387903	MK416107	MK416064
LaVe1	Lamium bifidum—receptacle	Ottaviano	MK387879	MK416083	MK416040
LaPo2	Lamium purpureum—receptacle	Portici	MK387877	MK416081	MK416038
MfCa2	Micromeria fruticulosa—gall wall	Capri	MK387882	MK416086	MK416043
MgPo1	Micromeria graeca—receptacle	Pontone	MK387890	MK416094	MK416051
MgLu1	Micromeria graeca—ovary	Lucrino	MK387918	MK416122	MK416079
MgLu2	Micromeria graeca—receptacle	Lucrino	MK387901	MK416105	MK416062
MgVi1	Micromeria graeca—gall wall	Vivara	MK387893	MK416097	MK416054
MgVi2	Micromeria graeca—larva of Asphondylia sp.	Vivara	MK387887	MK416091	MK416048
MgVi3	Micromeria graeca—receptacle	Vivara	MK387892	MK416096	MK416053
Nc/f17	Nepeta cataria—receptacle	Konopnica	MK387896	MK416100	MK416057
SpCa1	Salvia sp.—receptacle	Capri	MK387891	MK416095	MK416052
ThSC1	Thymus sp.—receptacle	Monte Santa Croce	MK387909	MK416113	MK416070
Th/S345	Thymus vulgaris—achene	Fajsławice	MK387889	MK416093	MK416050
Th/lg/2015	Thymus vulgaris—gall wall	Fajsławice	MK387912	MK416116	MK416073
Th/lg/2031	Thymus vulgaris—gall wall	Fajsławice	MK387897	MK416101	MK416058
Th/lg/2334	Thymus vulgaris—gall wall	Fajsławice	MK387894	MK416098	MK416055
Th/k/258	Thymus vulgaris—receptacle	Fajsławice	MK387895	MK416099	MK416056

2.2. Phylogenetic Analysis

Considering that recent work and revisions on the taxonomy of Cladosporium agree on the insufficient reliability of morphological characters for a correct species ascription [1,8,10], the selected isolates were directly processed for DNA extraction and sequencing of ITS, TEF1 and ACT regions. All the obtained DNA sequences listed in Table 2 have been deposited in GenBank, to be available for further taxonomic assessments.

Identification based on DNA sequencing and BLAST searches in GenBank showed that four strains could be ascribed to C. ramotenellum and three to C. allicinum, which are widespread saprobes within the C. herbarum s.c. [1]. However, the majority of the collected strains (33) were found to belong in the C. cladosporioides s.c., and were further analyzed for assessing their phylogenetic relationships with all the members of this taxonomic group. Overall, the phylogenetic analysis included 141 strains and was based on a nucleotide set of 1164 bp (536 bp for ITS, 373 bp for TEF1, and 255 bp for ACT).

The phylogram obtained through maximum likelihood (ML) analysis (Figure 1) shows that two strains from gall walls of Asphondylia nepetae can be respectively ascribed to C. delicatulum and C. perangustum, both known as saprobic and widely distributed species, while the remaining are grouped in four highlighted clades of the tree (A–D). The 16 isolates in group A are phylogenetically closely related to C. pseudocladosporioides (ML bootstrap/MP bootstrap/posterior probabilities = 92/88/1.0), with some exceptions. In particular, isolate Cl3 appears to be more closely related to C. crousii, while Th/K/258 and Th/lg/2334, two Polish isolates from Thymus vulgaris, form an independent clade (ML bootstrap/MP bootstrap/posterior probabilities = 87/87/1.0). The nine isolates in group B are phylogenetically closely related to C. cladosporioides (ML bootstrap/MP bootstrap/posterior probabilities = 96/82/1.0), with a certain degree of variation which is inferable from their distribution in several subclades. The two isolates in group C, collected in Campania from Micromeria graeca, form an independent clade in proximity to C. xylophilum (ML bootstrap/MP bootstrap/posterior probabilities = 100/100/1.0). Finally, the four isolates in group D result to belong to the same clade as C. europaeum (ML bootstrap/MP bootstrap/posterior probabilities = 100/100/1.0).

Figure 1

Phylogenetic tree based on maximum likelihood (ML) analysis of combined ITS, TEF1, and ACT sequences of 141 strains from the C. cladosporioides complex. Bootstrap support values ≥70% for ML and maximum parsimony (MP) are presented above branches as follows: ML/MP; bootstrap values <70% are marked with ‘-‘. Branches in bold are supported by Bayesian analysis (posterior probability >0.95). C. ramotenellum CPC 14300 was used as outgroup reference. Main clades are indicated by colored boxes A, B, C, and D.

2.3. Species Delimitation Assay

These four different groupings were separately analyzed along with the reference strains of the most closely related species by means of the automatic barcode gap discovery (ABGD) and general mixed Yule-coalescent (GMYC) methods for species delimitation. Results of these supplementary analyses were in agreement with one another, increasing the confidence of taxonomy assignments.

In detail, the set of strains forming group A was integrated by a reference strain for each of the six candidate species (Cladosporium sp. 3–8) which have been recently pointed out to exist within the C. pseudocladosporioides aggregate [7,8]. Besides the outgroup strain (C. hillianum), this overall set segregated in 13 taxa (Figure 2). The largest one is represented by 13 isolates, from both countries and miscellaneous origins, in association with the canonical reference strains of C. pseudocladosporioides, thereby confirming their belonging to this species sensu stricto. Moreover, an Italian isolate from Clinopodium vulgare (Cl3) matches with the representative of “Cladosporium sp. 5” (UTHSC DI-13-245), while two Polish isolates from T. vulgaris form an independent clade, which is close but separate from “Cladosporium sp. 7” (UTHSC DI-13-218).

Figure 2

Ultrametric tree phylogeny of group A showing results of sequence-based species delimitation methods. The tree is the result of a Bayesian analysis performed in BEAST on the concatenated ITS, TEF1, ACT dataset. For each node, posterior probabilities (if >0.90) are presented above the branch leading to that node. Results of species delimitation analyses through automatic barcode gap discovery (ABGD) and general mixed Yule-coalescent (GMYC) methods are congruent, as visualized by colored boxes to the right.

Likewise, considering the variation resulting in the general phylogenetic analysis, the set of strains in group B was integrated with six additional representatives of C. cladosporioides of which sequences are available in GenBank (Figure 3). In this case, the congruent analyses based on ABGD and GMYC indicate that 9 isolates of assorted origin in our sample are differentiated in 4 groups, each including at least one reference strain of C. cladosporioides.

Figure 3

Ultrametric tree phylogeny of group B showing results of sequence-based species delimitation methods. The tree is the result of a Bayesian analysis performed in BEAST on the concatenated ITS, TEF1, ACT dataset. For each node, posterior probabilities (if >0.90) are presented above the branch leading to that node. Results of species delimitation analyses through ABGD and GMYC methods are congruent, as visualized by colored boxes to the right.

Finally, the species delimitation analysis carried out for group C (Figure 4) indicates, with strong support, that the two isolates from receptacles of M. graeca represent an independent species, close to C. xylophilum, while the two couples of isolates from both countries included in group D cluster together with C. europaeum, confirming their ascription to this species (Figure 5).

Figure 4

Ultrametric tree phylogeny of group C showing results of sequence-based species delimitation methods. The tree is the result of a Bayesian analysis performed in BEAST on the concatenated ITS, TEF1, ACT dataset. For each node, posterior probabilities (if >0.90) are presented above the branch leading to that node. Results of species delimitation analyses through ABGD and GMYC methods are congruent, as visualized by colored boxes to the right.

Figure 5

Ultrametric tree phylogeny of group D showing results of sequence-based species delimitation methods. The tree is the result of a Bayesian analysis performed in BEAST on the concatenated ITS, TEF1, ACT dataset. For each node, posterior probabilities (if >0.90) are presented above the branch leading to that node. Results of species delimitation analyses through ABGD and GMYC methods are congruent, as visualized by colored boxes to the right.

2.4. Morphological Characteristics

Isolates showing significant divergence from known species of the C. cladosporioides s.c., thereby representing candidate novel species as revealed by the above mentioned phylogenetic and species delimitation analyses, were further examined with reference to their morphological and cultural characteristics. Morphological characters were evaluated in comparison to the phylogenetically most closely related species (Table 3). For the species related to C. xylophilum, some differences were observed consisting in shorter conidiophores and ramoconidia, a lower number of hila on the secondary ramoconidia, and slower growth on all culturing media. Based on evidence gathered from phylogenetic analyses and morphological examination, these candidate species are described as follows.

Table 3

Morphological characteristics of Cladosporium species novae described in this study.

Strains	Conidiophores (µm)	Ramoconidia (µm)	Secondary 1 Ramoconidia (µm)	Intercalary Conidia 1 (µm)	Conidia 1(µm)	Colony Diameter 2 after 14 Days (mm)
Th/lg/2334	(22−)70−130 × 2−3.6	12.9−36 × 2.5−4.1,0−1 septate	9.5−17.1 × 2.4−4	6.4−11 × 2−3.5	3−5.8(−6) × (1.5−)2−2.8	PDA: 63Malt-extract agar (MEA): 58Oatmeal agar (OA): 53
Th/k/258	(25−)42.7−151 × 2.4−5.1	14.3−39.8 × 2.4−5.2, 0−1 septate	7.9−23.2 × 2.6−4	5.6−8.8 × 2−3.9	3.8−5.6 × (1.5−)2−3	PDA: 70MEA: 53OA: 60
Cladosporium pseudocladosporioides [3]	15−155 × 2−4	19−48 × 3−4,0−2(−3) septate	16.1 × 2.9	8.8 × 2.6	4.1 × 2.1	PDA: 65−78MEA: 52−75OA: 55−73
MgPo1	(28.1−)44.4−142.5 × (2.1−)2.5−3.9(−4.5)	10.1−20.1 × 2.2−3.7 (−4.3)	(7.1−)8.3−14.6 × 2.1−3.1,2−4 apical hila	6.1−9.5 × 2−2.9	(2.1−)2.4−4.9(−5.1) × (1.7−)2.1−2.5(−2.8)	PDA: 47MEA: 37OA: 46
MgVi3	(57−)68−126.5 × (1.9−)2.4−4.2	11.5−22.2 × 2.4−3.5(−3.9)	(5.7−)7.4−16.6 × 1.8−2.72−4 apical hila	5.8−10.5 × 2−3.3	(1.4−)2.2−4.3 × (1.3−)1.6−2.5(−2.8)	PDA: 47MEA: 40OA: 45
Cladosporium xylophilum [3]	155(−190) × 2−4(−5)	19-35 × 2.5-3	14.5(±5.1) × 3.1(±0.5), up to 6(−9) apical hila	7.7(±2.2) × 2.6(±0.3)	3.9(±0.9) × 2.3(±0.3)	PDA: 52−74MEA: 47−74OA: 47−58

1 Average of 50 measurements. 2 Average of three replicates.

2.5. Taxonomy

Cladosporium polonicum Zimowska & Król sp. nov.—MycoBank MB839011; Figure 6.

Figure 6

Cladosporium polonicum Zimowska & Król sp. nov. (isolate Th/lg/2334, holotype). (a). Colony on PDA after 14 d; (b). colony on OA after 14 d; (c). colony on MEA after 14 d; (d–i). conidiophores and conidial chains; (e). tip of conidiophores and numerous conidia; (f). cylindrical-oblong, 0−1(−3) septate secondary ramoconidia and conidia; (g). tip of a conidiophore with several subdenticulate loci; (h–i). conidia.—Scale bars = 5 µm.

Similar to C. pseudocladosporioides, from which it differs in forming slightly shorter, 0−1 septate ramoconidia and shorter secondary ramoconidia.

Etymology: Named after the country where the representative strains were collected, Poland.

Mycelium immersed and superficial, hyphae unbranched or sparingly branched, up to 4 µm wide, septate, sometimes constricted at septa, subhyaline to pale olivaceous-brown, smooth or almost so, walls sometimes slightly thickened, sometimes irregular in outline due to swellings and constrictions, cells sometimes swollen, fertile hyphae minutely verruculose, mainly at the base of conidiophores. Conidiophores macronematous, sometimes also micronematous, solitary or in small loose groups, arising terminally and laterally from hyphae, erect, straight to slightly flexuous, cylindrical-oblong, non nodulose, sometimes once geniculate-sinuous or slightly swollen at the apex, unbranched or once branched, occasionally three times, branches often only as short denticle-like lateral outgrowth just below a septum, sometimes attenuated towards the apex, 0−5 septate, sometimes slightly constricted at septa, pale to pale medium olivaceous-brown, sometimes paler towards the apex, smooth or almost so, or asperulate or finely verruculose, walls slightly thickened or unthickened: (22−)42.7−151 × 2−3.6(−5.1) µm. Micronematous conidiophores filiform, narrower, not attenuated. Conidiogenous cells narrow, with 1−5 loci crowded at the apex, subdenticulate, 1−1.8 µm diam. Ramoconidia cylindrical-oblong, 0−1 septate pale olivaceous-brown, smooth, base broadly truncated, 2−3 µm wide, unthickened or slightly thickened, sometimes slightly refractive: 12.9−39.8 × 2.4−5.2 µm (av. 20.5 × 3.3). Secondary ramoconidia ellipsoid-ovoid to subcylindrical or cylindrical-oblong, 0−1(−3) septate, septum medium or often somewhat in the lower half, pale olivaceous to pale olivaceous-brown, smooth or almost so, sometimes slightly rough-walled, walls unthickened, with 1−4 distal hila, conspicuous, subdenticulate, somewhat thickened: 7.9−23.2 × 2.4−4 µm (av. 12.3 × 3.1). Microcyclic conidiogenesis not observed. Conidia very numerous, catenate, in branched chains, branching in all directions. Small terminal conidia obovoid, ovoid to limoniform or ellipsoid, sometimes subglobose, apex rounded or attenuated towards apex and base, 3−5.8 × (1.5−)2−3 µm, av. 5 × 2.2. Intercalary conidia ovoid, limoniform to ellipsoid or subcylindrical, 0(−1) septate, slightly attenuated towards apex and base, with 1−4 distal hila: 5.5−11 × 2−3.9 µm, av. 7.8 × 2.7.

Culture characteristics: Colonies on PDA attaining 63−70 mm diam after 14 days at 25 °C, olivaceous-grey, to grey olivaceous. Reverse leaden grey to olivaceous-black, felty-floccose, concentric ring visible in the center of colony, margin white very narrow up to 2 mm, glabrous, regular, aerial mycelium velvety to felty, growth flat, without exudates formed, sporulation profuse. Colonies on malt-extract agar (MEA) reaching 53−58 mm, grey olivaceous, reverse iron grey, floccose, margin white very narrow up to 2 mm, regular, glabrous, aerial mycelium velvety to felty, growth flat, without exudates, sporulation profuse, concentric ring visible in the center of colony. Colonies on oatmeal agar (OA) attaining 55−60 mm, olivaceous to grey olivaceous or olivaceous-buff, pale olivaceous-grey to greenish-grey towards margins. Reverse pale greenish-grey, leaden grey to iron grey, floccose, margin colorless up to 2 mm, glabrous, regular, aerial mycelium floccose to felty, radial sectors in the center of colony, sporulation profuse.

Specimens examined: POLAND, Lubelskie voivodeship, Fajsławice, from gall of Asphondylia serpylli Kieffer on thyme (Thymus vulgaris L., Lamiaceae), B. Zimowska, 18 June 2016, Th/lg/2334, holotype, preserved in a metabolically inactive state at the mycological collection of the Department of Plant Protection of the University of Life Sciences in Lublin; Konopnica, from receptacle in flower of catnip (Nepeta cataria L., Lamiaceae), B. Zimowska, 28 June 2018, Th/k/258.

Notes: Evidence resulting in a recent study [10] indicated C. crousii to be probably conspecific with C. pseudocladosporioides, also with reference to the very close species descriptions. Conversely, in our analysis, the species delimitation methods support both C. crousii and C. polonicum as separate species.

Cladosporium neapolitanum Zimowska, Nicoletti & Król sp. nov.—MycoBank MB839012; Figure 7.

Figure 7

Cladosporium neapolitanum Zimowska, Nicoletti & Król sp. nov. (isolate MgPo1, holotype). (a). Colony on PDA after 14 d; (b). colony on OA after 14 d; (c). colony on MEA after 14 d; (d–i). conidiophores and conidial chains; (d–e). macro- and micronematous conidiophores growing at an angle of 45−90°; (f). branched condiophore; (g). one septum secondary ramoconidium with broadly truncate base and four apical hila; (h–i). peculiar conidiogenesis characterized by sympodial proliferation of conidiogenous loci.—Scale bars = 5 µm.

Similar to C. xylophilum, from which it differs in forming shorter conidiophores, shorter ramoconidia and secondary ramoconidia, and for a lower number of hila at the apex of secondary ramoconidia.

Etymology: Named after the city of Napoli, Italy, in which surroundings the representative strains were collected.

Mycelium immersed and superficial, hyphae unbranched or loosely branched, 1−4(5) µm wide, septate, not constricted at septa, sometimes with irregular swellings and outgrowths, subhyaline to pale or medium olivaceous-brown, smooth to asperulate, minutely verruculose or irregularly verrucose, and rough-walled, with wart-like structures on the surface, walls unthickened, occasionally swollen at the base of conidiophores. Conidiophores macro- to sometimes micronematous, solitary, arising terminally and laterally from hyphae, erect, straight to slightly flexuous, cylindrical-oblong, usually neither nodulose nor geniculate, sometimes subnodulose at the uppermost apex, occasionally geniculate-sinuous, unbranched, sometimes once branched, 0−5 septate, sometimes slightly constricted at septa, pale to medium olivaceous-brown, smooth or almost so, sometimes somewhat irregularly rough-walled or verruculose, especially towards the base, sometimes wider at the base, or slightly toward the apex, walls slightly thickened: (28.1−)44.4−142.5 × 2.4−4.2 µm; growth sometimes proceeding at an angle 45−90°. Micronematous conidiophores paler, subhyaline to pale-olivaceous-brown, smooth or almost so. Conidiogenous cells terminal and intercalary, loci crowded at the apex forming clusters of pronounced scars, 2−5 conidiogenous loci formed at about the same level, loci often situated at lateral shoulders due to sympodial proliferation, loci 1−2 µm diam. Ramoconidia occasionally formed, cylindrical-oblong, 0(−1) septate, smooth, base broadly truncate 10.1−22.2 × 2.2−3.7(−4.3) µm. Secondary ramoconidia ellipsoid to cylindrical-oblong or irregular in outline, 0−1(−3) septate, septum median or somewhat in the upper half, not constricted, with 2−4 distal hila, crowded at the apex or situated on small lateral prolongations, pale olivaceous to pale medium olivaceous-brown, smooth or almost so, walls unthickened or almost so, hila conspicuous, subdenticulate to denticulate, (5.7−)7.4−16.6 × (1.4−)1.8−3.1 µm, av. 10 × 2.4. Conidia numerous, catenate, in densely branched chains, branching in all directions, straight. Small terminal conidia subglobose, obovoid, sometimes globose, aseptate, slightly attenuated towards apex and base, apex broadly rounded. Small terminal conidia and intercalary conidia almost smooth to often irregularly rough-walled, loosely verruculose to verrucose, attenuated towards apex and base, (1.7−)2.2−4.9 × 1.6−2.5(−2.8) µm, av. 3.5 × 2. Intercalary conidia ovoid, limoniform to ellipsoid or subcylindrical, sometimes irregular in outline, especially towards the distal end, due to numerous hila arranged in sympodial clusters of pronounced scars, 0−1 septate, septum median, not constricted, 5.8−10.5 × 2−3.3 µm, av. 7.7 × 2.5.

Culture characteristics: Colonies on PDA attaining 47 mm diameter after 14 days, pale green. Reverse iron-gray to brown-black, floccose to fluffy, margin white narrow up to 2−3 mm, slightly irregular, aerial mycelium abundant, velvety to floccose, loose to dense, growth flat, radial sectors visible in the center of colony, without exudates, sporulation profuse. Colonies on MEA reaching 37−40 mm, pale green. Reverse olivaceous to iron-black, velvety to floccose-felty, margin white narrow up to 2−3 mm, slightly irregular, aerial mycelium abundant, velvety to floccose, loose to dense, growth flat, radial sectors visible in the center of colony, without exudates, sporulation profuse. Colonies on OA reaching 45−46 mm, pale green paler in the center. Reverse iron-black, velvety to floccose-felty, margin white narrow up to 2−3 mm, slightly irregular, aerial mycelium abundant, velvety to floccose, loose, growth flat, radial sectors visible in the center of colony, without exudates, sporulation profuse.

Specimens examined: ITALY, Campania region, Pontone, from receptacle in flower of Micromeria graeca (L.) Benth. ex Rchb. (Lamiaceae), R. Nicoletti, 9 Apr. 2016, MgPo1, holotype, preserved in a metabolically inactive state at the mycological collection of the Department of Plant Protection of the University of Life Sciences in Lublin; isle of Vivara, from receptacle in flower of Micromeria graeca (L.) Benth. ex Rchb. (Lamiaceae), R. Nicoletti, 3 June 2016, MgVi3.

3. Discussion

Despite Cladosporium having been quite frequently reported as an associate in galls formed by Asphondyliinae on many plant species, so far, no attempts have been done to perform identification at the species level in order to ascertain whether or not these findings are to be referred to a definite species. In fact, symbiotic associations generally involve specific adaptations by the symbionts which are considered to characterize single or closely related taxa. Confirming this assumption, B. dothidea is now regarded as the fungal associate of these midges after some controversies occurred in the past which in most instances derived from nomenclatural reassessments [25,26]. This evidence obviously contrasts the hypothesis that Cladosporium may have a role in this peculiar biological association. Observations reported in the present study reinforce this conclusion, with reference to the degree of diversity which has been pointed out in the pool of Cladosporia recovered from galled and non-galled flowers of some species of Lamiaceae. In fact, our investigation carried out in two geographically distant areas demonstrated that (i) isolates of the same Cladosporium species can be recovered from both galled and non-galled flowers, and (ii) isolates from galls can be ascribed to at least seven species belonging to two species complexes.

Considering the uneven sampling with reference to both the plant species and the geographic areas, no definite association can be inferred. Within the C. herbarum s.c., the three strains of C. allicinum were all recovered from flower receptacles of Lamium and Lamiastrum spp., while the four strains of C. ramotenellum were found in flower receptacle of M. graeca and in galls of A. nepetae. Both these species are reported to be of worldwide occurrence in association with many heterogeneous plants [1].

Within the C. cladosporioides s.c., the species C. perangustum and C. delicatulum, both represented by single isolates from gall walls of A. nepetae, are known to be saprobic and widely distributed [27]. Two couples of isolates of C. europaeum were found on different species of Lamiaceae in Poland and Italy, which is to be taken as an indication of a more widespread occurrence in Europe of this species supporting its appropriately chosen name. In fact, it was recently separated from C. cladosporioides based on isolates from miscellaneous plant materials and indoor environments collected in Denmark, Germany, Portugal, and the Netherlands [10]; from the latter country, it has also been recovered from brown algae (Fucus sp.) [28]. With, respectively, 9 and 13 strains of assorted origin from both countries, C. cladosporioides and C. pseudocladosporioides are confirmed to be the most common representatives of this species complex. They both also show a notable degree of genetic variation, which is indicative of the possible existence of cryptic species, as predicted in previous studies and revisions [3,4,7,8,10]. In this respect, our phylogenetic study demonstrated correspondence of a strain from galls collected on C. vulgare to one of the candidate taxa, ‘Cladosporium sp. 5′, defined in the study by Sandoval-Denis et al. [7]. This strain and the two representatives of C. polonicum, which are also in phylogenetic proximity with C. pseudocladosporioides, might have been mistakenly ascribed to the latter species if the use of DNA sequences had been limited to a BLAST searches in the GenBank database. Hence, it is clear that in the absence of reliable morphological characters, the use of sequence-based statistical methods able to assess the significant phylogenetic distances is to be recommended in view of a correct classification, as well as to avoid the accumulation of misleading identifications of strains which have DNA sequences deposited in public repositories.

Even if displaying a certain degree of variation, many strains fitted in the cluster of C. cladosporioides. Our species delimitation analysis indicate that this grouping could be differentiated in four species, each including at least one strain from our sample and one reference strain, supporting the expectation that more new species could be separated within the currently defined C. cladosporioides. Considering that a more resolutive analysis should include most of the over 100 strains whose complete sets of sequences are available in GenBank, we decided not to try to get to more conclusive assessments in the present work, and to provisionally confirm identification of these Lamiaceae strains as C. cladosporioides.

With reference to the description of C. neapolitanum, it is interesting to consider that in their fundamental revision Bensch et al. [3] pointed out the existence of a certain degree of variation within C. xylophilum, and that the possible existence of cryptic species would have required to be ascertained based on a broader strain sample. Our finding seems to represent the first occasion meeting this expectation.

Besides emphasizing the need of a thorough revision of strains currently classified as C. cladosporioides and C. pseudocladosporioides, by the finding of two novel species our study confirms the taxonomic heterogeneity of the Cladosporium complex associated with flowers of Lamiaceae. Indeed, these plants represent a fruitful investigational ground for studying diversity of these ubiquitous fungi, also with reference to the possible contribution by endophytic strains to the biosynthesis of components of essential oils and other bioactive compounds, representing the basic property sustaining their industrial exploitation [29,30,31,32]. Interestingly, two isolates of each new species were found in two ecologically homogeneous areas in Poland and in Italy. Future investigations will disclose if they should be regarded as regional entities, or rather as more widespread taxa.

4. Materials and Methods

4.1. Isolates Collection

Cladosporium isolates considered in this study (Table 2) were recovered over 4 years (2015–2018) from several Lamiaceae species. Particularly, this sampling activity involved cropped T. vulgaris and a stand of N. cataria in Lubelskie voivodeship, south-eastern Poland, and species of Clinopodium, Micromeria, and a few additional taxa from several locations in Campania and Basilicata regions, southern Italy. A single isolate recovered from C. vulgare collected in Grunau im Almtal, Austria, was also included. Asphondylia galls were only found on Clinopodium nepeta, C. vulgare, Micromeria fruticulosa, M. graeca in Italy, and T. vulgaris in Poland, which implies that the isolates from the other species were all obtained from normal flowers. Isolation of fungal associates from gall walls and inquilines, that is midge larvae or their parasitoids, was carried out as specified in previous papers [23,24]. Isolations from the inner flower parts (receptacle, ovaries, or achenes developing inside the flower calyx) were carried out on potato-dextrose agar (PDA: Difco, Paris, France) amended with streptomycin sulphate (200 mg L−1), after dissecting the flowers with a sterilized scalpel in a laminar flow hood. All isolates were transferred in pure culture for taxonomic identification and storage in our in-house mycological collections.

4.2. DNA Isolation, Amplification and Sequencing

Selected strains were sampled from the surface of PDA cultures with a scalpel. The mycelial matter was transferred to 1.5 mL Eppendorf tubes for DNA extraction. DNA isolation was performed by means of a DNA easy plant and fungi isolation kit (EurX, Gdańsk, Poland), according to manufacturer’s protocol. DNA concentration was estimated on 1.5% agarose gel, compared with GeneRulerTM DNA Ladder Plus (Thermo Scientific, Waltham, MA, USA), and measured through a NanoDrop 2000 spectrophotometer (Thermo Scientific). DNA samples were diluted to a concentration of 20 ng µL−1 and stored at −20 °C. Amplification of loci currently considered in taxonomy of Cladosporium [4] was carried out using primers ITS1 and ITS4 for the rDNA-ITS region, primers EF1-728F and EF1-986R for the translation elongation factor 1-alpha (TEF1) region, primers ACT-512F and ACT-783R for the actin gene (ACT) [33]. PCR reaction mixtures, containing 20 ng of genomic DNA, 0.2 mM dNTP, 0.2 mM of each primer, 10 × Taq buffer (10 mM Tris-HCl, 1.5 mM MgCl2, and 50 mM KCl), and 1 U of Taq polymerase, were adjusted to a final volume of 25 µL with sterile distilled water. PCR was conducted in a Biometra T1 thermocycler (Analytik Jena, Jena, Germany). The following reaction profile was applied: 95 °C—5 min, 35 cycles (95 °C—45 s, 52 °C—45 s, and 72 °C—45 s), with final elongation at 72 °C—5 min. PCR products were separated in 1.5% agarose gels containing ethidium bromide in Tris/borate/EDTA buffer, at 140 V, for 1 h. After checking and determining the size of the resulting PCR products, samples were submitted for sequencing to Genomed (Warsaw, Poland).

4.3. Phylogenetic Analyses

The obtained nucleotide sequences were blasted in GenBank for a provisional species identification. Moreover, sequences of isolates belonging to the C. cladosporioides s.c. were submitted to a phylogenetic analysis including GenBank sequences of one or two strains for all the described species in this s.c. (Table 1). Strain CPC 14300 of C. ramotenellum, a species belonging to the C. herbarum s.c., was used as outgroup. The combined ITS, TEF1, and ACT sequences were aligned by using Muscle [34] and manually adjusted with AliView software [35], where necessary. Congruence between the different datasets was tested through the partition homogeneity test in PAUP software version 4.0b10 [36]. Gaps were treated as missing characters. The phylogenetic analyses were carried out in conformity with recent protocols [7,37]. The best nucleotide substitution model (generalized time-reversible model with gamma distribution and a portion of invariable sites (GTR+G+I) for the three independent data sets) was estimated using jModelTest version 2.3 [38] following the Akaike criterion. Phylogenetic analyses of the concatenated sequence data for maximum likelihood (ML) were performed by using RAxML software version 8.2.12 [39] with the GTR+G+I model of nucleotide substitution and 1000 bootstrap replications. Concatenated sequences were also analyzed for maximum parsimony (MP) by using PAUP, under the heuristic search parameters with tree bisection reconnection branch swapping, 100 random sequence additions, maxtrees set up to 1000, and 1000 bootstrap. Bayesian analyses were done with a Markov chain Monte Carlo (MCMC) coalescent approach implemented in BEAST 2 [40], using the uncorrelated lognormal relaxed clock, the GTR+G+I model, and a coalescent tree prior. Bayesian MCMC was run for 50 million generations, and trees and parameters were sampled every 1000 generations. The resulting log files were entered in Tracer v1.6.0 to check trace plots for convergence and effective sample size (ESS). Burn-in was adjusted to achieve ESS values of ≥ 200 for the majority of the sampled parameters. While removing a portion of each run as burn-in, log files and trees files were combined in LogCombiner. TreeAnnotator was used to generate consensus trees with 25% burn-in and to infer the maximum clade credibility tree, with the highest product of individual clade posterior probabilities. Phylogenetic trees were drawn by using FigTree software (tree.bio.ed.ac.uk/software/figtree/) (accessed on 10 December 2020). Both the alignments and the trees were deposited in Zenodo.

4.4. DNA-Based Species Delimitation

Four clades of the tree resulting from the general phylogenetic analysis were selected for DNA-based species delimitation analysis, in order to provide taxonomic assignment for our isolates. We explored two different delimitation methods, the automatic barcode gap discovery (ABGD) [41] and the general mixed Yule-coalescent (GMYC) model [42]. These methods are among the most popular approaches for species delimitation based on sequence data and are frequently used in studies on fungal diversity [43,44,45]. When several methods for species delimitation offer congruent estimates of species diversity, the confidence of taxonomy assignment for a given dataset increases [44]. The ABGD method was tested through a web interface (abgd web, bioinfo.mnhn.fr/abi/public/abgd/abgdweb.html) (accessed on 15 December 2020). Before analysis, the model criteria were set as follows: variability (P) between 0.001 (Pmin) and 0.1 (Pmax), minimum gap width (X) of 0.1, Kimura-2-parameters and 50 screening steps. To perform the GMYC delimitation method, an ultrametric tree was constructed in BEAST 2, as described above. After removing 25% of the trees as burn-in, the remaining trees were used to generate a single summarized tree in TreeAnnotator v.2.0.2 (part of the BEAST v.2.0.2 package) as an input file for GMYC analyses. The GMYC analyses with a single threshold model were performed in R (R Development Core Team, www.R-project.org) (accessed on 15 December 2020) under the “splits” package using the “gmyc” function (R-Forge, r-forge.r-project.org/projects/splits/) (accessed on 15 December 2020).

4.5. Morphological Observations

Morphological observations were carried out for strains representing candidate novel species. For the assessment of cultural characteristics, the isolates were grown on PDA, oatmeal agar (OA), and malt-extract agar (MEA, Difco), for 14 days at 24 °C in the dark. The colony right and reverse colours were rated according to the charts set up by Rayner [46]. Micromorphological observations were made from colonies grown for 7 days at 24 °C on synthetic nutrient-poor agar (SNA). Squares of transparent adhesive tape (Dalpo, Poznań, Poland) were placed on the sporulating areas at the colony margin. Observations were carried out under a BA 210 microscope (Motic, Xiamen, China), and images were taken through a 1 MP Motic camera and Scopelmage 9.0 software (Bioimager, Vaughan, Canada). From each isolate, minimum, maximum and mean values were measured for a set of relevant characters considered in taxonomy of this fungal genus [3]. Descriptions followed terminology used in Bensch et al. [1].