Skip to main content
Browse Subject Areas

Click through the PLOS taxonomy to find articles in your field.

For more information about PLOS Subject Areas, click here.

  • Loading metrics

Sequencing and Comparative Analysis of the Straw Mushroom (Volvariella volvacea) Genome

  • Dapeng Bao , (DPB); (QT)

    Affiliations National Engineering Research Center of Edible Fungi, Ministry of Science and Technology (MOST), Shanghai, P. R. China, Key Laboratory of Edible Fungi Resources and Utilization (South), Ministry of Agriculture, Shanghai, P. R. China, Institute of Edible Fungi, Shanghai Academy of Agricultural Sciences, Shanghai, P. R. China

  • Ming Gong,

    Affiliations National Engineering Research Center of Edible Fungi, Ministry of Science and Technology (MOST), Shanghai, P. R. China, Key Laboratory of Edible Fungi Resources and Utilization (South), Ministry of Agriculture, Shanghai, P. R. China, Institute of Edible Fungi, Shanghai Academy of Agricultural Sciences, Shanghai, P. R. China

  • Huajun Zheng,

    Affiliation Shanghai-MOST Key Laboratory of Health and Disease Genomics, Chinese National Human Genome Center at Shanghai, Shanghai, P. R. China

  • Mingjie Chen,

    Affiliations National Engineering Research Center of Edible Fungi, Ministry of Science and Technology (MOST), Shanghai, P. R. China, Key Laboratory of Edible Fungi Resources and Utilization (South), Ministry of Agriculture, Shanghai, P. R. China, Institute of Edible Fungi, Shanghai Academy of Agricultural Sciences, Shanghai, P. R. China

  • Liang Zhang,

    Affiliation Shanghai-MOST Key Laboratory of Health and Disease Genomics, Chinese National Human Genome Center at Shanghai, Shanghai, P. R. China

  • Hong Wang,

    Affiliations National Engineering Research Center of Edible Fungi, Ministry of Science and Technology (MOST), Shanghai, P. R. China, Key Laboratory of Edible Fungi Resources and Utilization (South), Ministry of Agriculture, Shanghai, P. R. China, Institute of Edible Fungi, Shanghai Academy of Agricultural Sciences, Shanghai, P. R. China

  • Jianping Jiang,

    Affiliation Shanghai-MOST Key Laboratory of Health and Disease Genomics, Chinese National Human Genome Center at Shanghai, Shanghai, P. R. China

  • Lin Wu,

    Affiliations National Engineering Research Center of Edible Fungi, Ministry of Science and Technology (MOST), Shanghai, P. R. China, Key Laboratory of Edible Fungi Resources and Utilization (South), Ministry of Agriculture, Shanghai, P. R. China, Institute of Edible Fungi, Shanghai Academy of Agricultural Sciences, Shanghai, P. R. China

  • Yongqiang Zhu,

    Affiliation Shanghai-MOST Key Laboratory of Health and Disease Genomics, Chinese National Human Genome Center at Shanghai, Shanghai, P. R. China

  • Gang Zhu,

    Affiliations National Engineering Research Center of Edible Fungi, Ministry of Science and Technology (MOST), Shanghai, P. R. China, Key Laboratory of Edible Fungi Resources and Utilization (South), Ministry of Agriculture, Shanghai, P. R. China, Institute of Edible Fungi, Shanghai Academy of Agricultural Sciences, Shanghai, P. R. China

  • Yan Zhou,

    Affiliation Shanghai-MOST Key Laboratory of Health and Disease Genomics, Chinese National Human Genome Center at Shanghai, Shanghai, P. R. China

  • Chuanhua Li,

    Affiliations National Engineering Research Center of Edible Fungi, Ministry of Science and Technology (MOST), Shanghai, P. R. China, Key Laboratory of Edible Fungi Resources and Utilization (South), Ministry of Agriculture, Shanghai, P. R. China, Institute of Edible Fungi, Shanghai Academy of Agricultural Sciences, Shanghai, P. R. China

  • Shengyue Wang,

    Affiliation Shanghai-MOST Key Laboratory of Health and Disease Genomics, Chinese National Human Genome Center at Shanghai, Shanghai, P. R. China

  • Yan Zhao,

    Affiliations National Engineering Research Center of Edible Fungi, Ministry of Science and Technology (MOST), Shanghai, P. R. China, Key Laboratory of Edible Fungi Resources and Utilization (South), Ministry of Agriculture, Shanghai, P. R. China, Institute of Edible Fungi, Shanghai Academy of Agricultural Sciences, Shanghai, P. R. China

  • Guoping Zhao,

    Affiliation Shanghai-MOST Key Laboratory of Health and Disease Genomics, Chinese National Human Genome Center at Shanghai, Shanghai, P. R. China

  •  [ ... ],
  • Qi Tan (DPB); (QT)

    Affiliations National Engineering Research Center of Edible Fungi, Ministry of Science and Technology (MOST), Shanghai, P. R. China, Key Laboratory of Edible Fungi Resources and Utilization (South), Ministry of Agriculture, Shanghai, P. R. China, Institute of Edible Fungi, Shanghai Academy of Agricultural Sciences, Shanghai, P. R. China

  • [ view all ]
  • [ view less ]


Volvariella volvacea, the edible straw mushroom, is a highly nutritious food source that is widely cultivated on a commercial scale in many parts of Asia using agricultural wastes (rice straw, cotton wastes) as growth substrates. However, developments in V. volvacea cultivation have been limited due to a low biological efficiency (i.e. conversion of growth substrate to mushroom fruit bodies), sensitivity to low temperatures, and an unclear sexuality pattern that has restricted the breeding of improved strains. We have now sequenced the genome of V. volvacea and assembled it into 62 scaffolds with a total genome size of 35.7 megabases (Mb), containing 11,084 predicted gene models. Comparative analyses were performed with the model species in basidiomycete on mating type system, carbohydrate active enzymes, and fungal oxidative lignin enzymes. We also studied transcriptional regulation of the response to low temperature (4°C). We found that the genome of V. volvacea has many genes that code for enzymes, which are involved in the degradation of cellulose, hemicellulose, and pectin. The molecular genetics of the mating type system in V. volvacea was also found to be similar to the bipolar system in basidiomycetes, suggesting that it is secondary homothallism. Sensitivity to low temperatures could be due to the lack of the initiation of the biosynthesis of unsaturated fatty acids, trehalose and glycogen biosyntheses in this mushroom. Genome sequencing of V. volvacea has improved our understanding of the biological characteristics related to the degradation of the cultivating compost consisting of agricultural waste, the sexual reproduction mechanism, and the sensitivity to low temperatures at the molecular level which in turn will enable us to increase the industrial production of this mushroom.


Volvariella volvacea, also known as the straw mushroom or Chinese mushroom, is an edible fungus that grows in tropical and subtropical regions. Most artificially cultivated straw mushrooms are produced in China where, in the 18th century, Buddhist monks of Nanhua Temple located in Guangdong Province enriched their diet by developing a primitive method that used fermented paddy straw as the growth substrate. The mushroom was held in such high regard that it was often presented as a tribute to Chinese royalty [1], [2].

In addition to rice straw, V. volvacea also grows on water-hyacinth, palm oil bunch wastes, pericarp wastes, banana leaves, and cotton waste [3]. Considered a health food because of its dietary and medicinal attributes [4], the mushroom is popular in southern China, Thailand, Malaysia and the Philippines. Previously ranked fifth among the major commercially-cultivated mushrooms [5], annual production of V. volvacea has increased in recent years due to a higher demand for health foods. In 2010, output of the mushroom on the Chinese mainland was 330,000 tons, accounting for more than 80% of global production.

Although V. volvacea has been cultivated for ∼300 years, multiple problems associated with the practice has greatly restricted development of the industry. The biological efficiency (conversion of the substrate into mushroom fruit bodies) of V. volvacea is only ∼15% on straw-based substrates and 30–40% on cotton-waste ‘composts’ [6], values which are considerably lower compared to other major cultivated species such as Agaricus bisporus, Lentinula edodes and Pleurotus spp. [3]. Furthermore, V. volvacea is a tropical fungus that requires relatively high temperatures (28–35°C) for vegetative growth and fruiting. Moreover, temperatures below 15 °C cause chilling damage to the fruiting body and adversely affect the viability of the fungal mycelia (Figure S1). Routine storage at low temperatures (4 °C) causes fruit body autolysis [7], thereby shortening mushroom shelf-life and hampering distribution over long distances.

V. volvacea has been described as a primary homothallic basidiomycete [1], [8], [9], whereby the homokaryotic mycelium arising from the germination of a single basidiospore is able to convert to the dikaryotic form and to complete the sexual cycle without mating (Figure 1). However, V. volvacea has multinucleate hyphae [10] and dikaryotic mycelia lack clamp connections, the morphological markers that differentiate the dikaryon from the homokaryon [11].

Figure 1. Life cycle and the fruiting body of Volvariella volvacea.

A. Basidiospores of V. volvacea are in tetrad and attached to a basidium by four sterigmata. Mature basidiospore germinates under favorable conditions to form primary mycelium. Secondary mycelia form by the fusion of primary mycelia, and give rise to fruiting bodies which create another new generation of basidiospore. The fruiting mycelium has no clamp connections. The life cycle of V. volvacea in general is complete in 4–5 weeks time [11], [90]. B. “Button” stages in the development of V. volvacea, which are harvested and sold in the market. C. A mature fruiting body.

We now report the complete genome sequence of the monokaryotic V. volvacea strain, V23-1. Our data will advance our understanding of the fungal cellulolytic system, thereby facilitating more efficient conversion of the agricultural wastes used as substrates for mushroom cultivation. Our transcript profiles from mycelia exposed to chilling will help identify factors regulating the sensitivity of this tropical fungus to low temperatures. Further research based on our results should also lead to recognition of the genetic determinants controlling sexuality in V. volvacea and the breeding of improved mushroom strains.

Results and Discussion

Genome sequencing and general features

The V. volvacea genome was sequenced using Roche 454 GS FLX and Illumina Solexa sequencing technologies. Combined sequences from the two technologies generated 190×coverage of the genome, and were assembled into 62 scaffolds with an N50 of 388 kb and a total genome size of 35.7 Mb (Table 1). The V. volvacea genome is similar in size to the genomes of several other species from the order Agaricales, including Schizophyllum commune (38.5 Mb) [12], Coprinopsis cinerea (37 Mb) [13] and P. ostreatus (35 Mb) [14], but larger than that of A. bisporus (30.2 Mb) [15].

Annotation of the assembled genome sequence generated 11,084 gene models, 76.43% of which are supported by Expressed Sequence Tag (EST) data. Approximately 9,370 (84.5%) gene models were assigned putative biological functions and the remaining 1,714 were hypothetical proteins and are presumed to be V. volvacea specific genes. Among the 11,084 gene models, 3,819 (34.5%), 1,995 (18.0%) and 1,617 (14.6%) were homologous to genes in Laccaria bicolor, C. cinerea and Serpula lacrymans var. lacrymans, respectively.

The average transcript length was 1,572 bp. Each gene contained an average of seven exons, with an average size of 229 bp, and introns with an average size of 88 bp (Table 1). Totally, 9,240 (83.4%) genes encoded proteins with homologous sequences in the NCBI nr protein databases, and 9,247 (83.4%) genes are mappable through the KEGG pathway database (Table 1).

An InterproScan analysis identified 2,103 conserved protein families in V. volvacea (containing 5,904 proteins) (Table S1), and KEGG analysis revealed 2,831 proteins involved in different pathways (Table S2). GO analysis assigned 5,161 proteins into different GO terms (Table S3). Altogether, 4,329 proteins were assigned to different KOG classes, and 2,518 protein domains were revealed in a total of 6,852 proteins (Table S4).

The genome encodes 824 secreted proteins and 1,681 transmembrane proteins (Table 1), indicating that 22.6% of encoded proteins are associated with the extracellular environment. The number of transfer RNA (tRNA) units was estimated to be 158 (Table S5). We observed 304 repeat units, with the total length of 2.25 Mb and occupying 6.18% of the entire genome, and 2,065 microsatellites (Table S6).

We observed a higher number of proteases (261) compared to other straw-rotting mushrooms such as A. bisporus (243) and C. cinerea (247) (Table S7). However, the number of protease families in these straw-rotting mushrooms (average 250 genes) was significantly smaller compared to the phytopathogenic fungi, Fusarium graminearum, Magnaporthe oryzae, Botrytis cinerea and Sclerotinia sclerotiorum (average 350 genes) and insect pathogenic fungi, Cordyceps militaris, Metarhizium anisopliae and M. acridum (average 390 genes) [16]. Representatives of the S01 trypsin subfamily, generally recognized to be virulence factors and pathogenicity markers [17], were absent in all straw-rotting mushrooms, suggesting that trypsin-like proteinases are not necessary for saprophytes [18]. The number of S08 subtilisin subfamily members, involved in the degradation of host cuticles and insect pathogenic fungal infections, was also smaller (11 on average among V. volvacea, A. bisporus, C. cinerea, and S. commune compared with 30 in insect pathogenic fungi). The number of M43 metallopeptidase subfamily members was significantly higher in V. volvacea (24) and C. cinerea (28) compared to just one in both phytopathogenic and insect pathogenic fungi [16]. Twenty-four V. volvacea M43 metallopeptidase genes were homologs of the P. ostreatus PoFE gene (E value<1.10e−22) expressed in mycelia [19] and the PoMTP gene (E value<2e−36) expressed in fruit bodies [20]. PoFE encodes a fibrinolytic enzyme with applicaton in thrombolytic therapy [19] while PoMTP plays an important role in the initiation and formation of mushroom fruit bodies [20].

Cytochrome P450 (CYP) plays various roles in fungi, including detoxification, degradation of xenobiotics and biosynthesis of secondary metabolites [21]. Similar to other basidiomycetes an average of 138 CYPs was observed in V. volvacea (Table S8). However, V. volvacea has the highest relative number of CYPs (1.24% of the total gene models) compared to other closely related mushroom species such as C. cinerea (1.00%), A. bisporus (1.11%) and S. commune (0.86%) (Table S8). Size of the fungal P450 could indicate an evolutionary history and adaptation to the environment [21]. CYP5136, CYP662, CYP665 and CYP 666 were present only in V. volvacea suggesting that the P450 family expanded in this fungus to meet the metabolic demand for biodegradation in various ecological niches (Table S9). Several fungal CYPs (i.e. CYP 58, 59, 60, 64, 65, 68, 505, 526), reported to be involved in the biosynthesis of aflatoxins, trichothecenes, and funonisins [22], [23], [24], [25] were not detected in V. volvacea. Other CYPs apparently lacking in V. volvacea and in some other basidiomycetes include CYP 56, essential for the formation of the outer spore wall layer in Saccharomyces cerevisiae and Candida albicans [26], [27], [28], (possibly indicating divergent biosynthetic pathway for spore wall formation in yeast and mushroom species), and CYP505, involved in fatty acid metabolism in Fusarium oxysporum [29], [30] (Table S9).

Phylogenomic analysis juxtaposing V. volvacea and 13 other fungi revealed closest evolutionary affinity with A. bisporus and C. cinerea (divergence time of 221 million years ago [MYA]) and S. commune (252 MYA) (Figure 2). The number of reductions in the V. volvacea gene families was 907, higher than the average number in other straw rotting fungi (567) and wood decay fungi (399) (Figure S2). This indicates that reduction in number of genes occurred during the evolution of V. volvacea. Interestingly, five large gene families (>160 genes) (in a total of 1,154 genes) were present in the V. volvacea genome, compared with 2 (452 genes) in A. bisporus, 3 (570 genes) in C. cinerea and 2 (655 genes) in S. commune (Figure S3). We suggest that functions of some gene families in V. volvacea may be enhanced during evolution for adaptation to specific growing niche. Furthermore, on a genomic scale, the percentage of amino acid sequence similarity was greater than 80% in only 257 pairs proteins in V. volvacea, virtually equal to the 255 pairs in C. cinerea, but much lower than 468 pairs in A. bisporus and 383 pairs in S.commune (Figure S4).

Figure 2. Phylogenomic tree showing the evolutionary distance of V. volvacea with different fungal species.

Rhizopus oryzae (zygomycete) was used as an outgroup. The topology of the phylogenomic tree was constructed by the neighbor-joining method [85] (bootstrap  = 1000, JTT matrix). All bootstrap values are 100%. Time scale was showed by MYA (million years ago). The divergence time of species is located on the right side of each node. The average deviation of divergence time for each node time is only 0.23 MYA.

Mating type locus and sexuality pattern

A Blastx scan of the V. volvacea V23-1 genome using basidiomycete homeodomain (HD) genes as the query, identified VVO_04854 and VVO_05004 genes (designated vv-HD1−V23−1 and vv-HD2−V23−1) located 271 bp apart on scaffold 07. Both encoded HD protein exhibiting a high similarity to homologs in the bipolar basidiomycetes, A. bisporus and Pholiota nameko, and tetrapolar basidiomycetes, C. cinerea and S. commune. It appears that V. volvacea has a single A mating type locus composed of two HD genes. Comparison of the genomic region flanking the V. volvacea A mating type locus with corresponding regions in A. bisporus, P. nameko and C. cinerea revealed a highly conserved synteny (Figure 3). When a pair of specific primers (VVmipF11 and VVmipR13), based on the sequence surrounding the mating type A locus in strain V23-1 (A1 locus), were used to amplify the A locus of the single-spore-isolate V23-18 (A2 locus), two genes, vv-HD1-V23−18 and vv-HD2-V23−18 (Accession number: JX157875) were identified within the A2 locus. These encoded HD1 and HD2 proteins that were 48% and 49% similar to the corresponding proteins from V23-1.

Figure 3. Comparison of the genomic structure of A mating type locus and its flanking region among C. cinerea, A. bisporus, V. volvacea and P. nameko.

Homologous genes are connected with lines. Arrows indicate the putative direction of transcription. Homeodomain protein genes (HD genes) are shown as red boxes. Green boxes indicate genes that are conserved among four species. Orange boxes indicate genes that are conserved among three species. Yellow boxes indicate genes that are conserved between two species. White boxes indicate genes that are not conserved among the four species. Data stem from C. cinerea (positions 2602748-2694125 from NCBI GenBank accession no. AACS02000001), A. bisporus (positions 862530-932075 from scaffold 1 in JGI Agaricus bisporus genome sequence,, V. volvacea (positions 379806-432904 from scaffold 7, HD1 position 406228–407814 and HD2 position 406060–404643) and P. nameko (positions 1734–39882 from NCBI GenBank accession no. AB435542).

Three genes, VVO_01536, VVO_09012 and VVO_09031 (designated vv-rcb1, vv-rcb2, vv-rcb3, respectively), located 72 and 4 kb apart on scaffold 24, were identified by Blast searches aimed at recognizing pheromone-receptor-like gene homologs. Deduced protein sequences of vv-rcb1, vv-rcb2 and vv-rcb3 genes were similar to other pheromone receptors and contained 7-transmembrane structures, which are characteristic of pheromone receptors in basidiomycetes with a mating type B locus [31]. However, although these data indicated a mating type B locus, the sequences of the putative locus and flanking region showed poor synteny when compared to other basidiomycetes. Furthermore, the genes encoding the pheromone precursor, which is required for the functioning of B mating factor [31], were not evident in the flanking region of the vv-rcb1, vv-rcb2 and vv-rcb3 genes. The DNA sequences of a second set of three pheromone-receptor-like genes, amplified using specific primes from a putative mating type B locus in strain V23-18 (which is compatible with V23-1), were identical to corresponding sequences in V23-1. Therefore, pheromone-receptor-like genes in V. volvacea may not regulate mating compatibility in the same way as in the bipolar fungi Coprinellus disseminatus [32] and P. nameko [33].

Molecular markers for A mating type genes were identified using two pairs of gene-specific primers (A1168F and A1168R for the A1 locus, and A2217F and A2217R for the A2 locus) designed according to the allelic sequences in mating type A locus. These markers can be used to distinguish homokaryotic and heterokaryotic single spore isolates (SSIs), and more effective than microscopic observations or SCAR (Sequenced Characterized Amplified Region) markers. A total of 124 SSIs derived from strain V23 were separated into three groups based on the presence of A1 and/or A2 locus as follows: A1 group (35 SSIs, 28.2%), A2 group (66 SSIs, 53.2%) and A1A2 group (23 SSIs, 18.6%). The 18.6% incidence of heterokaryons is higher than found among SSIs derived from V. volvacea strain Pingyou No. 1 (7.14%) [34] but considerably lower than reported among SSIs taken from strains H (77%, 23/30) and K (75%, 15/30) [9]. Long term artificial cultivation and/or a bigger test sample may account for the low incidence of heterokaryons among SSIs strains V23 and Pingyou No. 1. Nevertheless, the presence of both homokaryon and heterokaryon among SSIs derived from V23 is entirely consistent with previous observations [9], [34]. Furthermore, in accordance with earlier data obtained with the H and K strains of V. volvacea [9], cultivation tests undertaken in this study involving 12 SSIs assigned to the A1A2 groups and 14 designated homokaryotic SSIs confirmed that only the former were able to fruit. Of eight heterokaryons obtained by crossing SSIs belonging to the A1 and A2 groups, seven produced fruit bodies, indicating that the A mating type genes in V. volvacea regulate mating compatibility as in other mushrooms exhibiting bipolar sexual reproduction.

Phylogenetic analysis suggests that the bipolar HD proteins encoded by the A mating type genes in V. volvacea and other basidiomycetes originated from an ancestral HD protein associated with the tetrapolar basidiomycete, Ustilago maydis (Figure 4), supporting earlier claims [35], [36] that bipolar systems evolved from tetrapolar counterparts. The phylogenetic tree also indicated a close relationship between V. volvacea, A. bisporus, C. disseminatus and P. nameko. Loss of the B mating factor function in V. volvacea correlates with the inactivation of pheromone receptor-like genes [32], [37].

Figure 4. Phylogenetic tree constructed from the amino acid sequence alignments of homeodomain mating-type protein homologs of V. volvacea and various basidiomycete fungi.

Although V. volvacea has often been described as primary homothallic, this contention is still the subject of debate [38], [39], [40]. The phylogenetic data presented here support the notion that V. volvacea, like A. bisporus [41], is pseudo-homothallic. Such a system decreases the probability of out-breeding and increases the potential for inbreeding. This does not encourage genetic polymorphism, but ensures the high frequency of self-fertility and fruiting for effective transfer of genes required to flourish in a particular ecological niche (e.g. 30–35°C).

Carbohydrate active enzymes (CAZymes)

A total of 357 CAZyme-coding gene homologs were identified in the genome of V. volvacea more than the average (305) reported for several other basidiomycetes (Table S10). Of these, 224 homologs belong to the glycoside hydrolases (GH) superfamily, and respresented 42 families. Carbohydrate esterase (CE), glycosyl transferase (GT), polysaccharide lyase (PL) and carbohydrate-binding module (CBM) superfamilies were represented by 28, 66, 18 and 21 homologs respectively, distributed among 8, 24, 3 and 6 families, respectively (Figure 5, Table S10). The 18 PL models was the highest number recorded among several basidiomycetes. Analysis of CAZy families involved in plant polysaccharide degradation revealed 47, 101, and 57 candidate CAZymes related to the degradation of cellulose, hemicellulose and pectin, respectively in V. volvacea compared with the corresponding average values of 36, 77 and 37 for the other basidiomycetes (Figure 6, Table S11). V. volvacea also contained the highest number of putative β-1, 4-endoglucanases assigned to family GH 7 (14 compared with an average of 4 for other basidiomycetes), putative β-1,4-endoxylanases [42] belonging to family GH 10 (19, average 4), and putative pectin and pectate lyase (PL1) [42] (11, average 1). Interestingly, 30 putative GH 61 genes were detected in the genome, which is higher than the average found in other straw rotting fungi (C. cinerea and A. bisporus) (23), white rotting fungi (S. commune and P. chrysosporium) (18) and brown rotting fungi (P. placenta and S. lacrymans) (5). Recently, several GH 61 proteins have been shown to increase the activity of cellulases during lignocellulose degradation [43], [44]. The V. volvacea genome also contained a relatively large number of genes (57) encoding enzymes involved in the degradation of β-1,3-1,4-glucan, which are widely distributed as non-cellulosic matrix phase polysaccharides in cell walls of grasses and cereal species.

Figure 5. Comparison of the number of five CAZy genes in V. volvacea and other basidiomycetes fungi genomes.

Figure 6. Number of putative enzyme models involved in plant cell-wall degradation in V. volvacea and other basidiomycetes fungi genomes.

Fungal oxidative lignin enzymes

Although V. volvacea is generally regarded as a straw-degrading fungus, low substrate biological conversion rate have been attributed to an apparent lack of an efficient ligninolytic enzyme system [45], [46], [47]. Ligninolytic fungi degrade lignin using combinations of multiple isoenzymes of three heme peroxidases: lignin peroxidases (LiPs), manganese peroxidases (MnPs), and hybrid enzymes known as versatile peroxidases (VPs). The V. volvacea genome contains two putative MnP- and two putative VP-encoding genes, but lacks genes encoding LiPs (Table S12). In addition, 11 genes (vv-lac1 to vv-lac 11) encoding putative laccases, enzyme involved in various biological processes including lignin degradation, fungal development, melanin synthesis, and fungal pathogenesis of human and plant hosts [48], were also identified (Table S13). Six of these were identical to laccase genes isolated (by PCR using degenerate primers) in previous study [49], [50] (Table S13). The genomes of other straw-degrading mushrooms such as A. bisporus (12) and C. cinerea (17) also contain multiple laccase genes (Table S12). Ten of the eleven laccase genes in the V. volvacea genome were distributed through a 216 kb region in scaffold 6, and this gene cluster is supported by hypergeometric analysis. With the exception of vv-lac 11, all the other putative laccase genes were (when compared to A. bisporus and C. cinerea) clustered within a relatively short chromosomal region (Figure S5). Vv-lac 11 was located in scaffold 8 and closely resembles vv-lac6, possibly indicating a paralogous relationship (Figure S6A and Figure S6B). Phylogenetic analyses revealed that nine laccase genes (vv-lac1-5 and vv-lac7–10) are in the same cluster (Figure S6A). The locations of 17 out of 19 introns present in these nine laccase genes are conserved (Figure S6B), whereas, in C. cinerea the locations of only two out of 16 introns are conserved [51]. This might imply that the laccase genes in V. volvacea have derived from independent duplication-divergence events after speciation [52].

Although the functionality of individual laccase has yet to be confirmed, Chen et al. reported a significant increase in the expression of lac4 (vv-lac3 in this study) during pinhead formation, the first stage of fruit body development [50].

Transcriptional analyses of cold shock response

V. volvacea is unable to tolerate chilling injury resulting from contact with lower temperatures (above freezing), and exposure to 4 °C for more than eight hours causes irreversible damage leading to loss of viability [7]. High-throughput sequencing of mRNA expression in the vegetative hyphae exposed to 4 °C for 0, 2 and 4 h yielded 188999, 156430 and 191607 reads, respectively. Normalization of the data using DEGseq software disclosed that all the expressed genes participated in at least one of 270 metabolic pathways (Table S14). Comparison of the differences in gene expression levels between zero and 2 h, and zero and 4 h, using│log2 (fold-change)│> = 0.5 and FDR<0.001 as the threshold for significant changes, revealing 148 and 135 genes were up-regulated at 2 h and 4 h, respectively. The corresponding numbers of down-regulated genes were 117 and 153, respectively (Figure 7A, Figure 7B, and Table S15). Interestingly, 55 genes were both down-regulated at 2 and 4 h compared with only 25 up-regulated genes (Table S15). Among the 25 up-regulated genes, 19 were found to be conserved hypothetical proteins. VVO_05539 gene (log2 (0 H/2 H fold-change)  = 1.68, FDR = 0.0004; log2 (0 H/4 H fold-change) = 1.89, FDR = 5.77E−06) encodes a putative protein containing an F-box domain for protein-protein interaction that confers substrate specificity for ubiquitination. VVO_00268 gene (2.52, 1.19E−34; 2.60, 1.19E−41) encodes a putative protein with the conserved domain for the ubiquitin-conjugating enzyme E2. The inferred amino acid sequence of VVO_05394 (2.10, 4.51E−09; 4.07, 7.68E−77) gene shows a 71% identity and a 76% similarity with a senescence-associated protein in Picea abies (E value: 4e−56). Senescence-associated genes have generally been found to be up-regulated during leaf senescence, and the senescence-associated proteins such as RNases, proteinases, and lipases function as degradation enzymes [53], [54]. The inferred amino acid sequence of VVO_06566 (2.73, 0.00097; 3.27, 1.21E−06) gene contains the conserved domain for HNH (His-Asn-His) nucleases.

Figure 7. Differential gene expression in V. volvacea after exposure to 4 °C for different times.

Comparison of differentially expressed genes between 0 and 2 h (A), 0 and 4 h (B).

Among the 55 down-regulated genes at 2 and 4 h, 28 encode conserved hypothetical proteins. Eight of these (VVO_02676, VVO_07414, VVO_05796, VVO_05198, VVO_05208, VVO_09166, VVO_09167 and VVO_10542) are related to heat shock proteins (HSP) (Table S16). HSPs are reported to play an important role in protein folding when proteins are denatured due to oxidative stress, high pressure, and heat shock [55], [56], [57]. A number of HSP genes in Saccharomyces cerevisiae have been found to be induced between 6–48 h after exposure to temperatures as low as 4 °C [58]. HSPs in V. volvacea were down-regulated after exposure to 4 °C, although it remains unclear if this is connected to the higher sensitivity of the mushroom to lower temperatures.

Genes involved in trehalose and glycogen biosynthesis in yeast are induced after exposure to 4 °C [57], [59], suggesting that biosynthesis and accumulation of the reserve carbohydrates may be linked to cold tolerance and energy preservation [57]. Expression analysis of genes involved in starch and sucrose metabolism pathways (PATH: ko00500) revealed that 32 such genes were expressed at 0, 2 and 4 h following exposure to 4 °C (Figure S7, Table S17), although expression levels of the majority exhibited no significant change. Among them, VVO_02898 and VVO_08127, genes which encode the homologs of TPS 1 (trehalose-phosphate synthase) and TPS 2 (trehalose-6-phosphate phosphatase) in yeast, were repressed (−2.032, 9.01E−8) and no significant change at 2 h after exposure to 4°C. However, expression levels of TPS 1 and TPS 2 genes in S. cerevisiae were increased 5.6- and 5.9-fold respectively at 0°C [58], and 2- and 2.6-fold respectively at 4°C [57]. Genes involved in the glycolysis and gluconeogenesis pathways (PATH: ko00010) in V. volvacea was either repressed or showed no significant increase in expression after 2 and 4 hours exposure to 4°C (Figure S8, Table S18). These included VVO_06963 (encoding glyceraldehyde 3-phosphate dehydrogenase), VVO_03893 (encoding phosphoenolpyruvate carboxylkinase) and VVO_09324 (encoding aldehyde dehydrogenase family 7 member A1). Similarity, no significant increase in the expression of VVO_01210 (encoding stearoyl-CoA desaturase), VVO_00398 (encoding omega-6 fatty acid desaturase) and VVO_10684 (encoding acetyl-CoA acyltransferase 1), key genes involved in the biosynthesis of unsaturated fatty acids (PATH: ko01040), was observed following exposure to 4°C (Figure S9, Table S19). However, VVO_00127 (encoding 3-oxoacyl-[acyl-carrier protein] reductase, FabG) was expressed at 2 h (log2 (fold change) = 2.48, FDR = 7.22E−14), but not at 4 h (log2 (fold change) = 0.40, FDR = 0.56).

Although a variety of life forms indigenous to the tropics are unable to tolerate low temperatures, the underlying mechanisms are not well understood [60]. Exposure to low temperatures often triggers a common cold-shock response involving the biosynthesis of unsaturated fatty acids, accumulation of trehalose and glycogen, and the appearance of cold shock and heat shock proteins [61]. However, Li et al (1992) reported a significant decrease in the levels of unsaturation in V. volvacea membrane lipids at 0°C [62] and, while analysis of the V. volvacea genome revealed the presence of genes encoding enzymes involved in unsaturated fatty acids, trehalose and glycogen biosynthetic, the levels of gene over-expression recorded elsewhere was not evident. Thus, while biochemical adaptations and mechanisms that regulate low temperatures tolerance elsewhere have been described [61], these have yet to be elucidated in V. volvacea.

Sequencing of the V. volvacea genome provides a model for studying the evolution of specific molecular mechanisms associated with the saprophytic mode of nutrition, low temperature sensitivity and mating pattern exhibited by V. volvacea. Our data will serve as an information platform for future research directed at improved industrial production of this economically important edible mushroom.

Materials and Methods

Strains and culture conditions

The Volvariella volvacea dikaryotic strain, V23, which is widely cultivated in China, was provided by the Institute of Edible Fungi, Shanghai Academy of Agricultural Sciences. Twenty single spore isolates were obtained by spreading a suspension of basidiospores of strain V23 on Potato Dextrose Agar (PDA) plates (Becton, Dickinson, Sparks, USA) and confirmed as pure homokaryons by an inability to form sporophores under conditions that promoted fruit body formation by the dikaryotic parent. One of these, V23-1, was selected at random and used for genome sequencing.

Amplification of genes within the A mating type locus

The specific primer pair, VVmipF11 (5′-GTGACTGCTATGGAACACATTGGAC) and VVmipR13 (5′- TCGGAGGAAGCGGGTCCACTACA), was used to amplify the A mating type locus of V. volvacea. The two specific primer pairs, A1168F (5′-AGGGCATTCCAACCTATTCGCTTTC) and A1168R (5′-AATGTGAACAGTTTGAGCGGAGT), and A2217F (5′-GTGGTTGGGATGGAAGGTTGTGA) and A2217R (5′-CTGTGAGGGTTTGTGGTGGGATA), were used to amplify the A1 and A2 loci, respectively.

DNA extraction, genome sequencing, assembly and annotation

Genomic DNA was extracted from fungal mycelium using an improved cetyltrimethylammonium bromide (CTAB) method [63] as follows: freeze-dried mycelia (100 mg) was ground into a powder using a mortar and pestle and mixed with 1 mL CTAB buffer [2% CTAB, 1.4 M NaC1, 100 mM Tris HC1 (pH 8.0), 20 mM EDTA (pH 8.0)] preheated to 65°C. The homogenate was centrifuged (9650 g, 20 min, room temperature) and an equal volume of chloroform:isoamyl alcohol (24 1) added to the retained supernatant fraction. After gentle mixing, the suspension was kept at room temperature for 15 min and then centrifuged as above. The supernatant was transferred to a new microtube containing two-thirds volume of cold (−20°C) isopropanol and, after gentle shaking, the mixture was centrifuged (6450 g, 10 min, room temperature). The DNA pellet was washed three times with 1 mL 75% (v/v) ethanol (containing 10 mM potassium acetate), once with 1 mL cold 95% (v/v) ethanol, and air-dried. After dissolving the pellet in 50 µL TE buffer, RNA was removed by adding 1 µL RNase solution (10 mg/mL) and incubating at 37°C for 1 h. The DNA solution was then stored at −20°C until use.

The genomic DNA was sequenced using the Roche 454 GS FLX (Roche, USA) and Illumina Solexa GAIIx (Illumina, USA) platforms. Following pre-processing, the Roche 454 reads were assembled into a primary assembly using the Roche Newbler software and then scaffolds were constructed with Illumina paired-end and mate-pair reads using Velvet software (1.2.03) [64]. Gene model prediction was performed by combining four sets of software: GeneMark (2.8) [65], Augustus [66], FGENESH (2.6) [67] and GeneID (1.4.4) [68].The final gene model was determined with “GLAD”, an in-house developed automatic validation program that validated the final gene model employing gene length, EST frequency and annotation data. RepeatScout [69] and SciRoKo 3.4 software [70] was used to identify repetitive sequences and microsatellite sites in the genome, respectively.

RNA extraction, mRNA Purification, cDNA Synthesis, cDNA Sequencing

Fungal mycelium of V. volvacea strain V23 was grown in 250 mL flasks containing 100 mL Potato Dextrose Broth (PDB) (Becton, Dickinson, Sparks, USA) at 32 °C for 4 days, and then exposed to 4 °C for 0, 2 and 4 h. The treated mycelia were collected and lyophilized, and total RNA was extracted using Trizol reagent (Invitrogen, Carlsbad, USA) according to manufacturer's instructions. Double-stranded cDNA was synthesized from mRNA using the method of Ng et al with modifications [71]. A GsuI-oligodT primer and 1000 units of Superscript II reverse transcriptase (Invitrogen, Carlsbad, USA) were used to synthesize first-strand cDNA from 10 µg of mRNA. After incubation at 42 °C for 1 h, the 5′-CAP structure of mRNA was oxidized with NaIO4 (Sigma, USA) and ligated to biotin hydrazide. Biotinylated mRNA/cDNA was selected by binding to Dynal M280 beads (Invitrogen, Carlsbad, USA). After second strand cDNA synthesis, the polyA tail and 5′ adaptor were removed by GsuI digestion.

cDNA was size-calibrated using a cDNA size fractionation column (Agencourt), and fractions larger than 800 bp were sonicated to between 300–800 bp. These were then pooled together with other cDNA samples within the same size range, and transformed into single-stranded template DNA (sstDNA) libraries using the GS DNA Library Preparation kit (Roche Applied Science, USA). Libraries were clonally amplified in a bead-immobilized form using the GS emPCR kit (Roche Applied Science, USA) and sequenced with a 454 Genome Sequencer FLX system.

Identification of differentially expressed genes

The reads of three treated samples were separately mapped to predicted V. volvacea genes using BLASTN, and the expressed reads number of each gene was transformed into RPKM (Reads Per Kilobase per Million mapped reads) [72]. Differentially expressed genes were identified with the DEGseq package using the MARS (MA-plot-based method with Random Sampling) method [73]. A FDR ≤0.001 and an absolute value of log2Ratio ≥0.5 were adopted as threshold levels to assess the significance of contig expression difference.

Protein family classification and family size analysis

Whole genome protein families were classified by InterProScan [74] ( analysis and Pfam 26.0 [75] ( analysis. Protease families were additionally classified using Blastp against the MEROPS 9.7 peptidase database ( [76]. Cytochrome P450s were named according to the P450 database ( [77]. Transporters were classified based on the Transport Classification Database ( [78]. G-protein-coupled receptors were selected from the best hits to GPCRDB sequences ( tm/) [79]. Transcription factors were classified by Blastp searches against the Fungal Transcription Factor Database ( [80]. Protein kinases were classified by Blastp analysis against the KinBase database ( with a cutoff E value of 1e−15[81]. Carbohydrate-active enzymes (CAZymes) were classified by local Blastp searches against a library of catalytic and carbohydrate-binding module enzymes constructed from the CAZymes database ( [82]. To further study the distribution of lignin-modifying enzymes (LME) in fungal genomes, sequences of LME were extracted from the NCBI database. To build the LME database, our custom program compiled with perl was used to choose sequences based on the Blast results (Blastp, cut-off e-value >1e−50) from the obtained sequences. LME families were classified by Blastp against the LME database. Multigene families were generated from all the predicted proteins of selected genomes using SCPS tools [83] with default settings (Blastp, cut-off e-value >1e−30). The obtained multigene families were then analyzed for evolutionary changes in protein family size (>2) using the CAFE program [84].

Phylogenomic analysis and molecular clock estimation

Together with V. volvacea, 14 fungal species assigned mainly to the Basidiomycota (phyla are not italicized) and Ascomycota were used in the phylogenomic analysis. Genomic data for eight species (Agaricus bisporus, Aspergillus niger, Ganoderma lucidum, Phanerochaete chrysosporium, Puccinia graminis, Saccharomyces cerevisiae, Schizophyllum commune and Trichoderma reesei) were obtained from the Joint Genome Institute (JGI), and for five species (Coprinopsis cinerea, Cryptococcus neoformans, Neurospora crassa, Rhizopus oryzae, Ustilago maydis) from the Broad Institute. Single-copy orthologous protein sequences from the genomes of 14 species were obtained using our custom perl program. The tandem concatenated sequences consisting of 178 single-copy orthologous sequences from the 14 species were then used to construct a phylogenomic tree using the neighbor-joining method [85] (bootstrap  = 1000, JTT matrix). Timescale estimation of phylogenomic analysis with calibration was implemented in the codeml program [86] of the PAML package (version 4) [70]. The divergence time between species was estimated using PAML [87] by calibrating against the reassessed origin of U. maydis at 550 million years ago [88]. We used both global and local clock methods [89] to estimate the timescale of species divergence, and linear regression was applied to test the congruence between the global and local clocks.

Data availability and accession numbers

Data from this Whole Genome Shotgun project have been deposited at DDBJ/EMBL/GenBank ( under the accession number AMXZ00000000. The version described in this paper is the first version, AMXZ01000000. The transcript data have been deposited at NCBI SRA under the accession number: SRA061941.

Supporting Information

Figure S1.

Fruiting body of V. volvacea. (A). Fresh fruiting body. (B). Damaged fruiting body after exposure to 4 °C for 12 hours.


Figure S2.

The number of reductions in the gene families of V. volvacea and other basidiomycetes. The abbreviation: abis (Agaricus bisporus), ccin (Coprinopsis cinerea), cneo (Cryptococcus neoformans), gluc (Ganoderma lucidum), pchr (Phanerochaete chrysosporium), scom (Schizophyllum commune), umay (Ustilago maydis), and vvol (V. volvacea).


Figure S3.

Number of gene families in V. volvacea and other basidiomycetes.


Figure S4.

Distribution of paralogous genes with different levels of amino acid sequence similarity in V. volvacea and other basidiomycetes.


Figure S5.

Distribution of laccase genes in the genome of V. volvacea and other basidiomycetes.


Figure S6.

A. Neighbor joining tree of the deduced amino acid sequences of V. volvacea laccase gene. B. Intron positions within the laccase genes lac1-lac11 define two gene subfamilies. Black bars indicate intron positions. Dotted lines link the same introns.


Figure S7.

Heatmap showing expression levels of genes in starch and sucrose metabolism pathway at 0, 2 and 4 h after exposure to 4°C.


Figure S8.

Heatmap showing expression levels of genes in glycolysis and gluconeogenesis pathways at 0, 2 and 4 h after exposure to 4°C.


Figure S9.

Heatmap showing expression levels of genes in unsaturated fatty acid biosynthesis at 0, 2 and 4 h after exposure to 4°C.


Table S5.

The transfer RNA (tRNA) units in V. volvacea genome.


Table S6.

The microsatellite sites in V. volvacea genome.


Table S7.

Protease genes in different fungal genomes, arranged by MEROPS family.


Table S8.

The number and the relative ration of CYPs in basidiomycetes.


Table S9.

Cytochrome P450 (CYP) genes encoded in V. volvacea , C. cinerea , A. bisporus and S. commune genomes, arranged by CYP family.


Table S10.

Carbohydrate-degrading enzymes in V. volvacea and other basidiomycetes.


Table S11.

Comparative analysis of the number of CAZy families related to plant polysaccharide degradation in V. volvacea and other basidiomycetes.


Table S12.

The number of genes encoding the lignin oxidative enzymes in V. volvacea and other basidiomycetes.


Table S13.

The basic information of eleven laccase genes in V. volvacea genome.


Table S14.

The expressed genes in mycelia of V. volvacea during 4 °C exposure at 0 h, 2 h and 4 h.


Table S15.

The up-expression and down-expression genes in V. volvacea during 4 °C exprosure at 2 h and 4 h.


Table S16.

The expression of genes encoding the heat shock protein in V. volvacea during 4 °C exposure at 2 h and 4 h.


Table S17.

The genes expression of starch and sucrose metabolism pathway in V. volvacea during 4 °C exposure at 2 h and 4 h.


Table S18.

The genes expression of glycolysis and gluconeogenesis metabolism pathway in V. volvacea during 4 °C exposure at 2 h and 4 h.


Table S19.

The genes expression of unsaturated fatty acid biosynthesis pathway in V. volvacea during 4 °C exposure at 2 h and 4 h.



We thank Dr. Chengshu Wang for helpful comments, suggestions and manuscript reading, and Dr. John Buswell for linguistic revision.

Author Contributions

Conceived and designed the experiments: DPB GPZ QT. Performed the experiments: MJC HW YQZ LW GZ Y. Zhao. Analyzed the data: MG HJZ LZ JPJ Y. Zhou SYW. Contributed reagents/materials/analysis tools: DPB HW MG CHL. Wrote the paper: DPB MG HJZ.


  1. 1. Chang ST (1969) A cytological study of spore germination of Volvariella volvacea. Bot Mag 82: 102–109.
  2. 2. Chang ST (1977) The origin and early development of straw mushroom cultivation. Econ Bot 31: 374–376.
  3. 3. Chang ST (1974) Production of the straw mushroom (Volvariella volvacea) from cotton wastes. Mushroom J 21: 348–354.
  4. 4. Chang ST, Buswell JA (1996) Mushroom nutriceuticals. World J Microbiol Biotechnol 12: 473–476.
  5. 5. Chang ST (1996) Mushroom research and development - equality and mutual benefit. In: Royse DJ, editor,Mushroom biology and mushroom products.University Park, PA: Pennsylvania State University.pp. 1–10.
  6. 6. Chang ST (1980) Cultivation of Volvariella mushroom in Southeast Asia. Mushroom Newsletter for the Tropics 1: 5–13.
  7. 7. Chang ST (1978) Volvariella volvacea. In: Chang ST, Hayes WA, editors. The biology and cultivation of edible mushrooms. New York &London: Academic Press.pp. 573–603.
  8. 8. Chang ST, Chu SS (1969) Nuclear behaviour in the basidium of Volvariella volvacea. Cytologia 34: 293–299.
  9. 9. Chang ST, Yau CK (1971) Volvariella volvacea and its life history. Amer J Bot 58: 552–561.
  10. 10. Chang ST, Ling KY (1970) Nuclear behavior in the Basidiomycete, Volvariella volvacea. Amer J Bot 57: 165–171.
  11. 11. Chang ST (1965) A morphological study of Volvariella volvacea. Chung Chi Journal 5: 91–104.
  12. 12. Ohm RA, de Jong JF, Lugones LG, Aerts A, Kothe E, et al. (2010) Genome sequence of the model mushroom Schizophyllum commune. Nat Biotechnol 28: 957–963.
  13. 13. Stajich JE, Wilke SK, Ahren D, Au CH, Birren BW, et al. (2010) Insights into evolution of multicellular fungi from the assembled chromosomes of the mushroom Coprinopsis cinerea (Coprinus cinereus). Proc Natl Acad Sci USA 107: 11889–11894.
  14. 14. Ramírez L, Oguiza JA, Pérez G, Lavín JL, Omarini A, et al. (2011) Genomics and transcriptomics characterization of genes expressed during postharvest at 4°C by the edible basidiomycete Pleurotus ostreatus. Intl Microbiol 14: 111–120.
  15. 15. Morin E, Kohler A, Baker AR, Foulongne-Oriol M, Lombard V, Nagy LG, et al. (2012) Genome sequence of the button mushroom Agaricus bisporus reveals mechanisms governing adaptation to a humic-rich ecological niche. Proc Natl Acad Sci USA 109: 17501–17506.
  16. 16. Zheng P, Xia YL, Xiao GH, Xiong CH, Hu X, et al. (2011) Genome sequence of the insect pathogenic fungus Cordyceps militaris, a valued traditional chinese medicine. Genome Biology 12: R116.
  17. 17. Dunaevskii˘ IaE, Matveeva AR, Fatkhullina GN, Beliakova GA, Kolomiets TM, et al. (2008) Extracellular proteases of mycelial fungi as participants of pathogenic process. Russian J Bioorganic Chem 34: 317–321.
  18. 18. Kudryavtseva OA, Dunaevsky YE, Kamzolkina OV, Belozersky MA (2008) Fungal proteolytic enzymes: Features of the extracellular proteases of xylotrophic basidiomycetes. Microbiology 77: 643–653.
  19. 19. Shen MH, Kim JS, Sapkota K, Park SE, Choi BS, et al. (2007) Purification, characterization, and cloning of fibrinolytic metalloprotease from Pleurotus ostreatus mycelia. J Microbiol Biotechnol 17: 1271–1283.
  20. 20. Joh JH, Kim BG, Kong WS, Yoo YB, Kim NK, Park HR, Cho BG, Lee CS (2004) Cloning and developmental expression of a metzincin family metalloprotease cDNA from oyster mushroom Pleurotus ostreatus. FEMS Microbiol Lett 239: 57–62.
  21. 21. Črešnar B, Petrič Š (2011) Cytochrome P450 enzymes in the fungal kingdom. Biochim Biophys Acta 1814: 29–35.
  22. 22. Bhatnagar D, Ehrlich KC, Cleveland TE (2003) Molecular genetic analysis and regulation of aflatoxin biosynthesis. Appl Microbiol Biotechnol 61: 83–93.
  23. 23. Ehrlich KC, Chang PK, Yu J, Cotty PJ (2004) Aflatoxin biosynthesis cluster gene cypA is required for G aflatoxin formation. Appl Environ Microbiol 70: 6518–6524.
  24. 24. Yu J, Chang PK, Ehrlich KC, Cary JW, Bhatnagar D, Cleveland TE, Payne GA, Linz JE, Woloshuk CP, Bennett JW (2004) Clustered pathway genes in aflatoxin biosynthesis. Appl Environ Microbiol 70: 1253–1262.
  25. 25. Wen Y, Hatabayashi H, Arai H, Kitamoto HK, Yabe K (2005) Function of the cypX and moxY genes in aflatoxin biosynthesis in Aspergillus parasiticus. Appl Environ Microbiol 71: 3192–3198.
  26. 26. Briza P, Eckerstorfer M, Breitenbach M (1994) The sporulation-specific enzymes encoded by the DIT1 and DIT2 genes catalyze a two-step reaction leading to a soluble LL-dityrosine-containing precursor of the yeast spore wall. Proc Natl Acad Sci USA 91: 4524–4528.
  27. 27. Briza P, Kalchhauser H, Pittenauer E, Allmaier G, Breitenbach M (1996) N, N′-Bisformyl dityrosine is an in vivo precursor of the yeast ascospore wall. Eur J Biochem 239: 124–131.
  28. 28. Melo NR, Moran GP, Warrilow AG, Dudley E, Smith SN, Sullivan DJ, Lamb DC, Kelly DE, Coleman DC, Kelly SL (2008) CYP56 (Dit2p) in Candida albicans: characterization and investigation of its role in growth and antifungal drug
  29. 29. Nakayama N, Takemae A, Shoun H (1996) Cytochrome P450foxy, a catalytically self-sufficient fatty acid hydroxylase of the fungus Fusarium oxysporum. J Biochem(119): 435–440.
  30. 30. Kitazume T, Tanaka A, Takaya N, Nakamura A, Matsuyama S, Suzuki T, Shoun H (2002) Kinetic analysis of hydroxylation of saturated fatty acids by recombinant P450foxy produced by an Escherichia coli expression system. Eur J Biochem 269: 2075–2082.
  31. 31. Brown AJ, Casselton LA (2001) Mating in mushrooms: increasing the chances but prolonging the affair. Trends Genet 17: 393–400.
  32. 32. James TY, Srivilai P, Kues U, Vilgalys R (2006) Evolution of the bipolar mating system of the mushroom Coprinellus disseminatus from its tetrapolar ancestors involves loss of mating-type-specific pheromone receptor function. Genetics 172: 1877–1891.
  33. 33. Yi R, Tachikawa T, Ishikawa M, Mukaiyama H, Bao D, Aimi T (2009) Genomic structure of the A mating-type locus in a bipolar basidiomycete, Pholiota nameko. Mycol Res 113: 240–248.
  34. 34. Xie BG, Fu JS, Liu K (2010) Study on the genetics of Volvariella. volvacea. Annual Meeting for Mycological Society of China ,pp. 2–3.
  35. 35. Hibbett DS, Donoghue MJ (2011) Analysis of character correlations among wood decay mechanisms, mating systems, and substrate ranges in homobasidiomycetes. Syst Biol 50: 215–242.
  36. 36. Kües U, James TY, Heitman J (2011) Mating type in Basidiomycetes: unipolar, bipolar, and tetrapolar patterns of sexuality. The Mycota 14: 97–160.
  37. 37. Aimi T, Yoshida R, Ishikawa M, Bao DP, Kitamoto Y (2005) Identification and linkage mapping of the putative homeodomain protein (hox1) and the putative pheromone receptor homologue (rcb1) in a bipolar basidiomycete, Pholiota nameko. Curr Genet 48: 184–194.
  38. 38. Santiago CM (1983) Mycelial interaction and mating behavior in single spore isolates of Volvariella volvacea.. Philippines J Sci 114: 53–67.
  39. 39. Elliot TJ (1982) Genetics and breeding of cultivated mushrooms. In: Chang ST, Quimio, TH, editors.Tropical mushrooms: biological nature and cultivation methods.Hong Kong: The Chinese University Press. pp. 11–30.
  40. 40. Royse DJ, Jodon MH, Antoun GG, May BP (1987) Confirmation of intraspecific crossing and single and joint segregation of biochemical loci of Volvariella volvacea. Exp Mycol 11: 11–18.
  41. 41. Kerrigan RW (2011) Whole-genome sequencing of the cultivated button mushroom Agaricus bisporus: history, status, and applications. Proc 7th Intl Conf Mushroom Biology and Mushroom Products,pp. 1–6.
  42. 42. van den Brink J, de Vries RP (2011) Fungal enzyme sets for plant polysaccharide degradation. Appl Microbiol Biotechnol 91: 1477–1492.
  43. 43. Harris PV, Welner D, McFarland KC, Re E, Poulsen JC, et al. (2010) Stimulation of lignocellulosic biomass hydrolysis by proteins of glycoside hydrolase family 61: structure and function of a large, enigmatic family. Biochemistry 49: 3305–3316.
  44. 44. Sweeney MD, Xu F (2012) Biomass converting enzymes as industrial biocatalysts for fuels and chemicals: recent developments. Catalysts 2: 244–263.
  45. 45. Cai YJ, Buswell JA, Chang ST (1994) Production of cellulases and hemicellulases by the straw mushroom, Volvariella volvacea. Mycol Res 98: 1019–1024.
  46. 46. Buswell JA, Cai YJ, Chang ST, Peberdy JF, Fu SY, Yu HS (1996) Lignocellulolytic enzyme profiles of edible mushroom fungi. World J Microbiol Biotechnol 12: 537–542.
  47. 47. Chang SC, Steinkraus KH (1982) Lignocellulolytic enzymes produced by Volvariella volvacea, the edible straw mushroom. Appl Environ Microbiol 43: 440–446.
  48. 48. Giardina P, Faraco V, Pezzella C, Piscitelli A, Vanhulle S, Sannia G (2010) Laccases: a never-ending story. Cell Mol Life Sci 67: 369–385.
  49. 49. Chen SC, Ma D, Ge W, Buswell JA (2003) Induction of laccase activity in the edible straw mushroom, Volvariella volvacea. FEMS Microbiol Lett 218: 143–148.
  50. 50. Chen S, Ge W, Buswell JA (2004) Molecular cloning of a new laccase from the edible straw mushroom Volvariella volvacea.. FEMS Microbiol Lett 230: 171–176.
  51. 51. Kilaru S, Hoegger PJ, Kües U (2006) The laccase multi-gene family in Coprinopsis cinerea has seventeen different members that divide into two distinct subfamilies. Curr Genet 50: 45–60.
  52. 52. Lundell TK, Mäkelä MR, Hildén K (2010) Lignin-modifying enzymes in filamentous basidiomycetes-ecological, functional and phylogenetic review. J Basic Microb 50: 5–20.
  53. 53. Gan S, Amasino RM (1997) Making sense of senescence- Molecular genetic regulation and manipulation of leaf senescence. Plant Physiol 113: 313–319.
  54. 54. Espinoza C, Medina C, Somerville S, Arce-Johnson P (2007) Senescence-associated genes induced during compatible viral interactions with grapevine and Arabidopsis.. J Exp Bot 58: 3197–3212.
  55. 55. Godon C, Lagniel G, Lee J, Buhler JM, Kieffer S, Perrot M, Boucherie H, Toledano MB, Labarre J (1998) The H2O2 stimulonin Saccharomyces cerevisiae. J Biol Chem 273: 22480–22489.
  56. 56. Iwahashi H, Nwaka S, Obuchi K, Komatsu Y (1998) Evidence for the interplay between trehalose metabolism and Hsp104 in yeast. Appl Environ Microbiol 64: 4614–4617.
  57. 57. Pacheco A, Pereira C, Almeida MJ (2009) Small heat-shock protein Hsp12 contributes to yeast tolerance to freezing stress. Microbiology 155: 2021–2028.
  58. 58. Murata Y, Homma T, Kitagawa E, Momose Y, Sato MS, et al. (2006) Genome-wide expression analysis of yeast response during exposure to 4oC. Extremophiles 10: 117–128.
  59. 59. Kandror O, Bretschneider N, Kreydin E, Cavalieri D, Goldberg AL (2004) Yeast adapt to near freezing temperatures by STRE/Msn2,4-dependent induction of trehalose synthesis and certain molecular chaperones. Mol Cell 13: 771–781.
  60. 60. An D, Yang J, Zhang P (2012) Transcriptome profiling of low temperature-treated cassava apical shoots showed dynamic responses of tropical plant to cold stress. BMC Genomics 13: 64.
  61. 61. Aguilera J, Randez-Gil F, Prieto JA (2007) Cold response in Saccharomyces cerevisiae: new functions for old mechanisms. FEMS Microbiol Rev 31: 327–341.
  62. 62. Li Y, Cho KY, Wu YZ, Nair NG (1992) The effect of lipids and temperature on the physiology and growth of Volvariella volvacea.. World J Microbiol Biotechnol 8: 621–626.
  63. 63. Zhang H, Qin LH, Tan Q, Pan YJ (2006) Extraction of genomic DNA from Lentinula edodes using the CTAB Method. Journal of Shanghai University (Natural Science Edition) 12: 547–550.
  64. 64. Zerbino DR, Birney E (2008) Velvet: algorithms for de novo short read assembly using de Bruijn graphs. . Genome Res 18: 821–829.
  65. 65. Lomsadze A, Ter-Hovhannisyan V, Chernoff Y, Borodovsky M (2005) Gene identification in novel eukaryotic genomes by self-training algorithm. Nucleic Acids Research 33: 6494–6506.
  66. 66. Mario S, Burkhard M (2005) AUGUSTUS: a web server for gene prediction in eukaryotes that allows user-defined constraints. Nucleic Acids Research 33: W465–W467.
  67. 67. Salamov AA, Solovyev VV (2000) Ab initio gene finding in Drosophila genomic DNA. Genome Res 10: 516–522.
  68. 68. Parra G, Blanco E, Guigó R (2000) GeneID in Drosophila. Genome Res 10: 511–515.
  69. 69. Price AL, Jones NC, Pevzner PA (2005) De novo identification of repeat families in large genomes. Bioinformatics 21: I351–I358.
  70. 70. Robert Kofler, Christian Schlötterer, Tamas Lelley (2007) SciRoKo: A new tool for whole genome microsatellite search and investigation. Bioinformatics 23: 1683–1685.
  71. 71. Ng P, Wei CL, Sung WK, Chiu KP, Lipovich L, Ang CC, Gupta S, Shahab A, Ridwan A, Wong CH, Liu ET, Ruan Y (2005) Gene identification signature (GIS) analysis for transcriptome characterization and genome annotation. Nat Methods 2: 105–111.
  72. 72. Mortazavi A, Williams BA, McCue K, Schaeffer L, Wold B (2008) Mapping and quantifying mammalian transcriptomes by RNA-Seq. Nat Methods 5: 621–628.
  73. 73. Wang L, Feng Z, Wang X, Wang X, Zhang X (2010) DEGseq: an R package for identifying differentially expressed genes from RNA-seq data. Bioinformatics 26: 136–138.
  74. 74. Quevillon E, Silventoinen V, Pillai S, Harte N, Mulder N, Apweiler R, Lopez R (2005) InterProScan: protein domains identifier. Nucleic Acids Res 33: W116–W120.
  75. 75. Finn RD, Mistry J, Tate J, Coggill P, Heger A, et al. (2010) The Pfam protein families database. Nucleic acids research 38: D211–D222.
  76. 76. Rawlings ND, Barrett AJ, Bateman A (2012) MEROPS: the database of proteolytic enzymes, their substrates and inhibitors. Nucleic Acids Res 40: D343–D350.
  77. 77. Nelson DR (2009) The Cytochrome P450 Homepage. Human Genomics 4: 59–65.
  78. 78. Saier MH Jr, Tran CV, Barabote RD (2006) TCDB: the Transporter Classification.
  79. 79. Vroling B, Sanders M, Baakman C, Borrmann A, Verhoeven S, Klomp J, Oliveira L, de Vlieg J, Vriend G (2011) GPCRDB: information system for G protein-coupled receptors. Nucleic Acids Res 39: D309–D319.
  80. 80. Park JS, Park JJ, Jang SW, Kim SY, Kong SH, et al. (2008) FTFD: An Informatics Pipeline Supporting Phylogenomic Analysis of Fungal Transcription Factors. Bioinformatics. 24: 1024–1025.
  81. 81. Natarajan K, Taylor S, Zhai Y, Venter C, Manning G (2007) Structure and function of the microbial kinome. PLoS Biol 5: e17.
  82. 82. Cantarel BL, Coutinho PM, Rancurel C, Bernard T, Lombard V, Henrissat B (2009) The Carbohydrate-Active EnZymes database (CAZy): an expert resource for Glycogenomics. Nucleic Acids Res 37: D233–238.
  83. 83. Paccanaro A, Casbon JA, Saqi MA (2006) Spectral clustering of protein sequences. Nucleic Acids Res 34: 1571–1580.
  84. 84. De Bie T, Cristianini N, Demuth JP, Hahn MW (2006) CAFE: a computational tool for the study of gene family evolution. Bioinformatics 22: 1269–1271.
  85. 85. Saitou N, Nei M (1987) The neighbor-joining method: a new method for reconstructing phylogenetic trees. Mol Biol Evol 4: 406–425.
  86. 86. Goldman N, Yang Z (1994) A codon-based model of nucleotide substitution for protein-coding DNA sequences. Mol Biol Evol 11: 725–736.
  87. 87. Yang Z (2007) PAML 4: phylogenetic analysis by maximum likelihood. Mol Biol Evol 24: 1586–1591.
  88. 88. Martin F, Aerts A, Ahrén D, Brun A, Danchin EG, et al. (2008) The genome of Laccaria bicolor provides insights into mycorrhizal symbiosis. Nature 452: 88–92.
  89. 89. Yang Z, Yoder AD (2003) Comparison of likelihood and Bayesian methods for estimating divergence times using multiple gene loci and calibration points, with application to a radiation of cute-looking mouse lemur species. Syst Biol 52: 705–716.
  90. 90. Chang ST (1966) Spore of Volvariella volvacea. Nature 212: 528–529.