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Genomic content of a novel yeast species Hanseniaspora gamundiae sp. nov. from fungal stromata (Cyttaria) associated with a unique fermented beverage in Andean Patagonia, Argentina

  • Neža Čadež,

    Roles Conceptualization, Funding acquisition, Investigation, Methodology, Writing – original draft

    Affiliation Biotechnical Faculty, University of Ljubljana, Jamnikarjeva 101, Ljubljana, Slovenia

  • Nicolas Bellora,

    Roles Data curation, Formal analysis, Methodology, Software, Validation, Visualization, Writing – review & editing

    Affiliation Laboratorio de Microbiología Aplicada y Biotecnología, Instituto de Investigaciones en Biodiversidad y Medio-ambiente, Consejo Nacional de Investigaciones, Científicas y Técnicas (CONICET)-Universidad Nacional del Comahue, Bariloche, Argentina

  • Ricardo Ulloa,

    Roles Methodology, Resources

    Affiliation Laboratorio de Bioprocesos, Instituto de Investigación y Desarrollo en Ingeniería de Procesos, Biotecnología y Energías Alternativas, Consejo Nacional de Investigaciones, Científicas y Técnicas (CONICET)-Universidad Nacional del Comahue, Neuquén, Argentina

  • Chris Todd Hittinger,

    Roles Conceptualization, Investigation, Validation, Writing – review & editing

    Affiliation Laboratory of Genetics, Genome Center of Wisconsin, DOE Great Lakes Bioenergy Research Center, Wisconsin Energy Institute, J. F. Crow Institute for the Study of Evolution, University of Wisconsin-Madison, Madison, Wisconsin, United States of America

  • Diego Libkind

    Roles Conceptualization, Funding acquisition, Investigation, Resources, Supervision, Validation, Writing – review & editing

    Affiliation Laboratorio de Microbiología Aplicada y Biotecnología, Instituto de Investigaciones en Biodiversidad y Medio-ambiente, Consejo Nacional de Investigaciones, Científicas y Técnicas (CONICET)-Universidad Nacional del Comahue, Bariloche, Argentina


A novel yeast species was isolated from the sugar-rich stromata of Cyttaria hariotii collected from two different Nothofagus tree species in the Andean forests of Patagonia, Argentina. Phylogenetic analyses of the concatenated sequence of the rRNA gene sequences and the protein-coding genes for actin and translational elongation factor-1α indicated that the novel species belongs to the genus Hanseniaspora. De novo genome assembly of the strain CRUB 1928T yielded a 10.2-Mbp genome assembly predicted to encode 4452 protein-coding genes. The genome sequence data were compared to the genomes of other Hanseniaspora species using three different methods, an alignment-free distance measure, Kr, and two model-based estimations of DNA-DNA homology values, of which all provided indicative values to delineate species of Hanseniaspora. Given its potential role in a rare indigenous alcoholic beverage in which yeasts ferment sugars extracted from the stromata of Cytarria sp., we searched for the genes that may suggest adaptation of novel Hanseniaspora species to fermenting communities. The SSU1-like gene encoding a sulfite efflux pump, which, among Hanseniaspora, is present only in close relatives to the new species, was detected and analyzed, suggesting that this gene might be one factor that characterizes this novel species. We also discuss several candidate genes that likely underlie the physiological traits used for traditional taxonomic identification. Based on these results, a novel yeast species with the name Hanseniaspora gamundiae sp. nov. is proposed with CRUB 1928T (ex-types: ZIM 2545T = NRRL Y-63793T = PYCC 7262T; MycoBank number MB 824091) as the type strain. Furthermore, we propose the transfer of the Kloeckera species, K. hatyaiensis, K. lindneri and K. taiwanica to the genus Hanseniaspora as Hanseniaspora hatyaiensis comb. nov. (MB 828569), Hanseniaspora lindneri comb. nov. (MB 828566) and Hanseniaspora taiwanica comb. nov. (MB 828567).


Since the introduction of DNA sequence analysis for species delineation, the number of newly described species of the yeast genera Hanseniaspora and Kloeckera (the allied anamorphic genus) has increased from seven to nineteen [16]. A similar number of newly described species can be observed for other yeast genera, mostly as an extensive database of barcode sequences of D1/D2 and internal transcribed spacer (ITS) regions provides data of all described species [7]. However, additional protein-coding genes have also been employed in yeast taxonomy to construct statistically well-supported phylogenetic trees that reflect the evolutionary relationships among species and genera [810]. With emergence of whole genome sequencing, reconstructions of more robust yeast phylogenies are now being recovered [1114], from which a frame for new species definition is being built [1521]. A shift from phenotype- to sequence-based taxonomy enables introduction of the new International Code of Nomenclature for algae, fungi, and plants (Shenzhen Code; [22]) by which the teleomorphic genus Hanseniaspora has a priority over its anamorphic counterpart, Kloeckera, by the rules of nomenclature and the number of species assigned to each genus [23]. Accordingly, the three asexual species Kloeckera hatyaiensis, Kloeckera lindneri and Kloeckera taiwanica should be transferred to the genus Hanseniaspora (see Taxonomy).

Ecologically, yeasts belonging to the genus Hanseniaspora are the most common of the apiculate yeasts. They are found on various fruits, flowers, and bark as their primary habitat. Insects may also serve as their dispersal vectors, and the soil may serve as their reservoir [24,25]. The main sources of simple sugars in the environment include the decaying fruits on which Hanseniaspora species predominate and fruiting bodies, such as those of Cyttaria hariotii, a fungal parasite of Nothofagus, a tree endemic to Southern hemisphere forests. During maturation, C. hariotii stromata become rich in fermentable sugars, a substrate typical for yeast communities in which Hanseniaspora species often becomes prevalent [16,2628]. However, the availability of simple sugars from ripe fruits is short-term, which is suggesting that apiculate yeasts mostly reside in soil or are associated with other plant material [29]. For Hanseniaspora species, these habitats are also consistent with their assimilation profiles because they can utilize only those few carbon sources that are available in tree bark, such as cellobiose, arbutin, and salicin [30]. Additionally, Hanseniaspora yeasts have unusually high vitamin requirements [31], which further suggests their close association with plant material.

During the exploration of the biodiversity of fermenting yeast communities in the stromata of the tree fungus C. hariotii in Andean Patagonia [27,3233], we found two apiculate yeast strains that were distinct from known species. DNA sequence comparisons of rRNA- and protein-coding genes suggested that they represent a novel yeast species, which is described here as Hanseniaspora gamundiae sp. nov. We also provide a draft genome sequence and analysis of Hanseniaspora gamundiae CRUB 1928T to accompany the formal description of the new species. Interestingly, genome content correlates with several physiological traits and suggests possible adaptations of this species to its ecological niche.

Materials and methods

Yeast isolation and physiological characterization

The two strains examined in this study were isolated from the stromata of C. hariotii of Nothofagus dombeyi (“Coihue”) and of Nothofagus antarctica collected from the Andean forests of Patagonia, Argentina (S1 Table). The Argentinean National Park Administration issued a permission for sampling. Stromata were processed as described by Libkind et al. [27] and Sampaio and Gonçalves [34], respectively. Strain CRUB 1604 was isolated using selective media of Yeast Nitrogen Base (YNB, Difco) supplemented with 1% (w/v) raffinose and 8% (v/v) ethanol and purified on Yeast Malt Agar (YMA). Strain CRUB 1928T was isolated without any carbon source in the media, although pieces of C. stromata, which naturally contain simple sugars, were added as an inoculum. The strains were phenotypically characterized by standard methods, including assimilation tests conducted in liquid media for 3 weeks at 26°C [35]. Sporulation was investigated on 5% malt agar (Difco; Becton, Dickinson and Company) at 26°C over 3 weeks.

Phylogenetic placement

The MasterPure Yeast DNA Purification kit (Epicentre) was used to extract DNA from cultures grown on yeast extract-peptone-glucose agar (YPD, Sigma) plates for 2 days. Amplification of DNA sequences encoding the internal transcribed spacer (ITS, 657 bp), the large subunit rRNA (LSU) D1/D2 domain (571 bp), actin (encoded by ACT1, 949 bp), and translation elongation factor-1a (EF-1α, encoded by TEF1, 695 bp) was performed as described by Cadez et al. [36]. These DNA sequences were determined by a commercial sequencing facility (Macrogen Inc., The Netherlands).

The dataset of ITS-D1/D2-actin-EF-1α sequences generated during this study, along with the previously determined sequences of the related species [2], were aligned using the MUSCLE algorithm [37] and concatenated. Phylogenetic relationships were inferred by the Maximum Likelihood (ML) method using the substitution model of Tamura-Nei [38] with gamma-distribution rates (G) calculated in MEGA6 [39]. Bootstrap support [40] was determined from 1,000 pseudoreplicates. Conflicting topologies of single gene ML trees were determined by using Consensus Network algorithm (threshold 0.1) as implemented in program SplitsTree 4.14 [41]. Parsimony network analysis was performed using the aligned ITS-D1/D2 sequences, excluding gaps at 95% connection limit with the program TCS 1.21 [42].

PCR fingerprinting

To examine the genetic relatedness between the proposed new species and its closest relatives, genomic fingerprinting using three microsatellite primers ((ATG)5, (GTG)5, and (GACA)4) was used in PCR amplification reactions, as described previously [43]. Similarities between the combined fingerprints were calculated using the Pearson’s product moment correlation coefficient (r), based on the overall densitometric profiles of the banding patterns. Cluster analysis of the pairwise values was performed using the UPGMA algorithm as implemented in the BioNumerics 7.5 computer program.

Preparation of library for sequencing genomic DNA

For genome sequencing, Hanseniaspora gamundiae strain CRUB 1928T was cultured in 15 ml YM broth [35] for 72 h at 26°C. DNA was extracted as described by Bellora et al. [44]. About 5 μg of gDNA was sonicated and ligated to Solexa sequencing adaptors (Illumina) using the manufacturer’s kit [45]. The paired-end library was sequenced by using the Illumina HiSeq 2000 and MiSeq in accordance with the manufacturer’s instructions.

Genome assembly and annotation

De novo genome assembly was performed with SPAdes 3.9.0 [46] with options -m 60 -t 20. A total of 6,841,738 paired-end reads from five sequencing sets with mean lengths of 145, 96, 95, 96, and 94 nt and estimated insert sizes of 369, 332, 356, 163, and 333 nt, respectively, yielded 6722 contigs. These contigs were merged into 338 scaffolds longer than 2000 bp with median read coverage of 29.3. Read coverage was used to estimate the ratio between single-copy nuclear, mitochondrial, and rDNA regions. Reads were aligned to the ITS/5.8S region, D1/D2 region, ACT1, and TEF1 of the Hanseniaspora gamundiae sp. nov. CRUB 1928T genome with Blat v34 [47] using the default parameters (NCBI accession numbers KU674841, KU674853, KU674865, and KU674877, respectively).

Simple repeats and transposable elements were identified by RepeatMasker v4.0.3 [48] using the RepBase database [49]. Only those repetitive elements with more than 100 occurrences were considered. tRNAs were predicted by tRNAscan-SE v1.23 [50]. GeneMark-ES v2.3e [51] was used for gene prediction (parameters: -min_contig 8000 –max_nnn 1000). Coding sequences (CDSs) were retrieved by recording the Reciprocal BLAST Best Hits (e-value < 10−5, identity > 50%) against the Saccharomyces cerevisiae (SGD) proteome [52] as a reference and to the proteome of the Hanseniaspora vineae T02-19AF (NCBI) genome predicted with GeneMark-ES v2.3e [51] using the same parameters as above. All predicted genes were annotated by using Blast2GO 3.3 [53].

Phylogenomic analyses

Similarities between the genomes were calculated using an alignment-free matching algorithm with a DNA seed based on 9 bases (110110101000111), as implemented in BioNumerics 7.6. Subsequent clustering using these similarity values enabled phylogenomic placement of H. gamundiae. The level of genomic sequence divergence between closely related species was estimated using the Kr value, an alignment-free pairwise distance measure calculated with Genome Tools [54]. The calculations of Average Nucleotide Identity (ANI) values were performed by web-based calculator available at [55]. We also estimated DNA–DNA homology (DDH) values with the Genome-to-Genome Distance Calculator (GGDC) 2.1 provided by the DSMZ web site ( The DDH values presented here were calculated using Formula 2, which estimates DDH values based on the identities of high-scoring segment pairs (HSPs) [56].

Assigning genes to enzyme functions

Predicted protein sequences were assigned an enzyme function using TBLASTN and BLASTP searches using query protein sequences from the characterized pathways in the model organism Saccharomyces cerevisiae S288c against subject databases built from the Hanseniaspora genome assemblies. We used Best reciprocal hits (BRH) relying on BLASTP hits (e-value threshold of 10−5) to estimate the presence of each gene.


The electronic version of this article in Portable Document Format (PDF) in a work with an ISSN or ISBN will represent a published work according to the International Code of Nomenclature for algae, fungi, and plants, and hence the new names contained in the electronic publication of a PLOS article are effectively published under that Code from the electronic edition alone, so there is no longer any need to provide printed copies.

In addition, new names contained in this work have been submitted to MycoBank from where they will be made available to the Global Names Index. The unique MycoBank number can be resolved and the associated information viewed through any standard web browser by appending the MycoBank number contained in this publication to the prefix The online version of this work is archived and available from the following digital repositories: PubMed Central, LOCKSS.

Results and discussion

Species delineation and phylogenetic placement

While studying the diversity of native fermenting yeasts from natural Andean forests in Patagonia, Argentina, in particular that of Saccharomyces spp., we studied approx. 600 samples of bark, soil and Cyttaria stromata along all Andean Patagonia [16,3233]. The frequency of yeasts in those samples averaged 70%, of which ca. 54% were Saccharomyces spp. either S. eubayanus or S. uvarum [33]. Other frequent species were Kregervanrija spp., Kregervanrija delftensis, Torulaspora af. delbrueckii, Torulaspora microellipsoides, Zygosaccharomyces cidrii, Lachancea nothofagi. Among those were two apiculate yeast strains (S1 Table). We sequenced and analyzed the genes encoding the ITS/5.8S and LSU D1/D2 domains of rRNA and the actin and translation elongation factor-1α (EF-1α) proteins. The two isolates shared identical D1/D2 LSU and actin gene sequences, while they differed by two nucleotides each in the ITS and in the EF-1α datasets (strains CRUB 1604 and CRUB 1928T). A BLAST similarity search with the D1/D2 LSU revealed that the apiculate yeasts belonged to the genus Hanseniaspora and that these sequences did not have an exact match in the GenBank. Their nearest match was to the type strain of H. taiwanica (EF653942) with 5 substitutions. This phylogenetic placement was also statistically well supported (bootstrap 100%) by phylogenetic analysis of the concatenated gene sequences encoding ribosomal rRNA, actin, and EF-1α (Fig 1A). Because the classical guidelines for species delineation introduced by Kurtzman and Robnett [57] may be overly conservative for closely related Hanseniaspora species [36], we identified interspecific discontinuity by parsimony haplotype network analysis of the concatenated ITS and D1/D2 sequences, as suggested by Lachance et al. [58]. At the 95% connection limits, haplotypes of the two Argentinian strains investigated in this study formed a parsimony network separated from H. taiwanica (69 missing links in 1210 bp dataset), indicating the genetic isolation of both taxa (Fig 1B). This differentiation was further confirmed by pairwise comparisons between strain CRUB 1928T of the new species and the neighboring type strain of H. taiwanica in their D1/D2, ITS, ACT1, and TEF1 datasets. As shown in Fig 1A, the percentage of sequence divergences in protein-coding genes (ACT1 and TEF1) exceeded 3%, which we consider indicative of two closely related but distinct species of Hanseniaspora [1]. However, the pairwise distances of 12.2% in the ITS region differed widely from the pairwise distances of 0.9% in the LSU D1/D2 region between Argentinian strains and H. taiwanica (Fig 1A). These findings further confirm heterogeneities in the evolutionary rates of genetic regions; compared to the majority of ascomycetous yeasts, ITS regions evolve unusually quickly, while D1/D2 regions are unusually conserved in Hanseniaspora species [36,57]. As such conflicting signal can lead to a less accurate phylogeny [11, 59] we reconstructed the relationship between H. gamundiae and its closest relatives also in form of a phylogenetic network (Fig 1C). It confirmed previously determined relationships (Fig 1A) between these species excluding presence of conflicting phylogenetic signals. Nevertheless, the restricted number of the strains studied may hamper the estimation on intraspecific variation.

Fig 1. Placement of Hanseniaspora gamundiae sp. nov. within the genus Hanseniaspora based on the sequences of the ITS and the D1/D2 LSU regions of the gene encoding the rRNA, as well as the genes encoding actin and elongation factor-1α (EF-1α) proteins.

(A) A phylogenetic tree inferred using Maximum-Likelihood analysis based on the Nei-Tamura model in MEGA6 [39]. Bootstrap analysis was carried out with 1000 pseudoreplicates [40]; only values above 50% are shown. Wickerhamomyces anomalus was used as the outgroup. Bar, nucleotide substitutions per site. p, indicating percentage of substitutions between the two marked sequences for each of the four individual genes or p-distance. (B) Parsimony networks based on the ITS and D1/D2 LSU of the rRNA gene sequences of strains of H. gamundiae sp. nov. and its closest relative H. taiwanica. Each connecting line represents a single nucleotide substitution, and each small circle indicates a missing intermediate haplotype. The rectangle indicates the sequences identified as ancestral by the analysis. Analyses were performed using TCS 1.21 [42]. (C) A consensus network showing relationships between H. gamunidae and its closest relatives. H. mollemarum [6] is not included in phylogenetic analyses.

The genetic divergence of the strains belonging to the novel species was confirmed by PCR fingerprinting as well. The PCR-fingerprints of the strains CRUB 1604 and CRUB 1928T segregated them from their closest relatives (S1 Fig). Based on the data presented above, we propose a novel yeast species, Hanseniaspora gamundiae sp. nov. (MycoBank no. MB824091), to accommodate these strains within the genus Hanseniaspora.

Genome analysis

De novo genome assembly of Hanseniaspora gamundiae type strain CRUB 1928T yielded a 10.2-Mbp genome assembly with a coverage of 29.3-fold, which was assembled into 338 scaffolds with shortest scaffold at the 50% of genome length of 63 kb, and with 0.46% of unknown bases (Table 1).

Table 1. Comparative analysis of genomes, assemblies, and gene statistics for Hanseniaspora gamundiae sp. nov. and other Hanseniaspora species.

The G+C content of the new species’ genome is 37.1%, which is similar to the genomes of H. vineae [60] and H. osmophila [61]. The latter two species have the highest G+C values known for Hanseniaspora species, whether measured by exact calculations from the genome sequencing (Table 2) or estimated by thermal denaturation (an approach whose estimates were generally from 1.5 to 3% higher [62]). Of the 4,624 predicted genes, 4,452 were cannonical protein-coding genes (96.3%, Table 2). As introduced by Bellora et al. [44], by using the excess sequencing coverage of contigs for the mitochondrial genome (mtDNA) and rDNA loci, we estimated the copy number ratio of mtDNA per nDNA as 883:1 and the rDNA locus per nDNA as 77:1 in the genome of H. gamundiae CRUB 1928T (Table 2).

Next, the phylogenetic markers LSU D1/D2, ITS/5.8S, EF-1α, and actin (KU674858, KU674846, KU674882K, and KU674870, respectively) were aligned to the genome sequences of the same strain. The number of mismatches in genome assembly was low as there was only one to two nucleotide differences in sequences determined by Sanger sequencing. Repeat and low complexity sequences cover 2.7% of the genome and, of those, 27% are represented by transposable elements (TEs). TEs present in more than 100 copies per genome were classified [63] as LTR retrotransposons corresponding to Gypsy/Ty3 and Copia/Ty1, LINE elements corresponding to Jockey and L1 of non-LTR retrotransposons, and hAT superfamilies corresponding to DNA cut-and-paste transposons. Most of these elements are widespread in the family Saccharomycetaceae [64].

Annotated genes of H. gamundiae were mapped against de novo-predicted genes of H. vineae T02/19AF and genes of S. cerevisiae S288c from Saccharomyces Genome Database using the reciprocal best BLAST hit algorithm. The majority of the 3451 genes (74.6%) were shared by all three species, and only a small proportion was specific to either the closely related H. vineae or the distantly related S. cerevisiae: 8% and 6.7%, respectively (Table 2). Recently, Shen et al. [13] reported on the low coverage of H. valbyensis and H. uvarum genes (62.2% and 64.5%, respectively) from the BUSCO set of 1438 single-copy, conserved fungal genes, suggesting accelerated evolutionary rates or pervasive gene loss in these genomes. Nevertheless, for H. vineae, which is closely related to H. gamundiae but more distantly related to H. valbyensis and H. uvarum, this phenomenon was not observed. For H. gamundiae, we found 242 out of the 248 highly conserved set of core eukaryotic genes (CEG) proposed by Parra et al. [65], suggesting that H. gamundiae is also not a victim of accelerated evolution or pervasive gene loss.

Genomic diversity

The genome of H. gamundiae CRUB 1928T was compared to the genomes of six out of nineteen Hanseniaspora species (Table 1) and to distantly related species of the family Saccharomycetaceae using an alignment-free matching algorithm. As shown in Fig 2 and S2 Table, the species placement agreed with the tree based on the concatenated ribosomal RNA and protein-coding genes (Fig 1).

Fig 2. Phylogenomic relationships of the nine Hanseniaspora strains based on an alignment-free matching algorithm with a nine bases DNA seed.

Saccharomyces cerevisiae and Kluyveromyces lactis were used as outgroups. Similarities among closely related genomes are presented as the Alignment-Free Distance Measure (Kr), Average Nucleotide Identity (ANI) and by estimating digital DNA-DNA Homology values (dDDH values).

The genome similarities among closely related species were estimated using an alignment-free distance measure, Kr [54]. H. gamundiae and its closest sequenced relative, H. vineae, share Kr values of 0.2, a value previously shown by Bellora et al. to correspond to distinct species [44]. However, the Kr values are somewhat lower for the comparison of the closely related taxa of H. vineae and H. osmophila, which share intermediate DNA-DNA reassociation values (45–60%, [62]). Since boundaries between Hanseniaspora species were originally set using DNA-DNA reassociation measurements, we estimated DNA-DNA homology values (DDH) between Hanseniaspora genomes by using Average Nucleotide Identity (ANI) calculator [55] and Genome-to-Genome Distance Calculator (GGDC, [56]). The highest scores using ANI calculator were among closely relates species pairs H. guilliermundii-H. opuntiae and H. vineae-H. osmophila which is in agreement with previous conclusions based on DNA-DNA reassociation values of 35% and 33%, respectively [36,62]. However, the dDDH values were higher only among the closely related H. vineae-H. osmophila species pair (53%). On the other hand, H. gamundiae had lower similarity scores (19.7%-30%) when compared to all other Hanseniaspora genomes. Both approaches proved useful for providing indicative values to delineate species of Hanseniaspora.

Habitat and possible adaptation to fermenting communities

Both strains of the novel species Hanseniaspora gamundiae were isolated during our survey of fermentative yeasts colonizing obligate biotrophic stromata of Cyttaria spp. (Ascomycota, Leotiomycetes, Cyttariales) and the bark of its host trees, Nothofagus spp., suggesting the new yeast species is associated with this niche. Its closest known relative is the recently described species of H. taiwanica [4], whose three strains were isolated from fruiting bodies of different mushrooms in Taiwan. These are the only reports of isolations of Hanseniaspora species from mushrooms, making it difficult to infer them as their fundamental niche. Standard physiological profiles for these species also do not reveal a clear picture. The main carbon sources found in stromata are the sugar alcohol mannitol, the disaccharide trehalose, and the polysaccharides glycogen and chitin [66], none of which can be assimilated by either H. gamundiae or H. taiwanica suggesting their dependence on other community members [67]. However, the sugar composition of mature C. hariotii consists of up to 10.2% of the simple sugars of fructose, glucose, and sucrose [68,69], which resembles the composition of grape juice, a substrate in which Hanseniaspora species predominate.

The Mapuche tribe, whose traditional territory is coincident with the Nothofagus forests in Patagonia, collected and consumed Cyttaria stromata in many ways, some of which continue to the present [70]. Similar to the many cereals, fruits, and roots fermented by people elsewhere, natives of this tribe used this fungus to produce an alcoholic fermented beverage (called chicha) from these sugar-rich stromata [71]. The Cyttaria beverage could have been obtained by squeezing fresh stromata and collecting the resulting juice, which fermented spontaneously, or simply by leaving the entire stromata in cooled boiled water for a few days [72]. Several yeasts inhabit Cyttaria stromata in their various maturation stages [16,28], although most are not likely to have contributed much to the distinctive properties of chicha. Given that both strains of H. gamundiae were isolated in the late maturation stages of stromata as part of a fermenting microbiota and given that Hanseniaspora spp. play a significant role in sugar fermentation and flavor generation during wine production [73,74], we speculate that H. gamundiae could have been a major player in the initial stages of traditional chicha fermentation. Much as occurs during the spontaneous wine fermentation with communities rich in S. cerevisiae, we further speculate that chicha fermentations may have been traditionally outcompeted at later stages by Saccharomyces uvarum and/or Saccharomyces eubayanus [16,27,28].

In this context, we searched the genome sequence of H. gamundiae for genes that may provide advantages during mixed species fermentation. One such gene encodes a sulfite efflux pump (SSU1); among Hanseniaspora species with available genome sequences, SSU1 is present only in H. gamundiae and its closest relatives, H. vineae and H. osmophila, (Table 1). Saccharomyces spp. produce sulfite in the presence of fermentable sugars and under nitrogen-limiting conditions, and this compound arrests the growth of sulfite-sensitive yeasts in mixed communities [75,76]. However, the functionality of SSU1 was not verified in this study.

Detailed investigation of the organization of the SSU1 locus in Hanseniaspora spp. (Fig 3) revealed that the SSU1 gene is adjacent to a gene encoding a NAPDH dehydrogenase (OYE2-like), whose S. cerevisiae homolog is involved in oxidative stress response. This arrangement is reminiscent of the linkage between SSU1 and GLR1, which encodes a glutathione reductase, in the genome of S. cerevisiae [77,78]. Interestingly, compared to S. cerevisiae, H. gamundiae has a conserved gene order and an unusually high sequence identity of those genes that are in proximity of the SSU1 gene. However, instead of a gene encoding a sulfite efflux pump, it harbors the DTR1 gene, which encodes a putative dityrosine transporter that is expressed during sporulation [79]. Similar synteny conservation has also been reported for some representatives of the family Saccharomycetaceae, such as Eremothecium assybii, Kluyveromyces lactis, and a group of European Saccharomyces paradoxus strains that harbor a second copy of SSU1 of unknown origin next to DTR1 [80,81]. During the diversification of Hanseniaspora, genomic rearrangements may have resulted in different positions for the SSU1 gene within the genome, but its conservation may have been key for the success of some Hanseniaspora spp. in habitats like the sugar-rich stromata of Cytarria that are rich in fermenting competitors. Nevertheless, due to the seasonal occurrence of mature Cyttaria stromata, they might represent only a transient habitat for H. gamundiae, and SSU1 conservation may also be important in surrounding niches, including immature Cyttaria, insects, tree bark, or the soil underneath trees.

Fig 3. Schematic gene organization around the putative sulfite pump gene SSU1 (purple) in H. gamundiae sp. nov. and related species.

Green arrows indicate genes without synteny, while the color intensity of arrows from yellow (40–50% nucleotide similarity), to orange (80–90% similarity), to red (more than 90% similarity), indicate the level of conservation between orthologous genes. Gene sizes and distances are approximately to scale. Numbers in parentheses indicate scaffold number and location of genes in the assembled genome.

Physiological characteristics of H. gamundiae and their correlation to the genome content

Similar to other Hanseniaspora species, H. gamundiae is characterized by a limited set of growth abilities, which precludes the use of conventional physiological tests for its identification. H. gamundiae can be distinguished from its sibling species, H. taiwanica, only by its inability to assimilate glucono δ-lactone, while it can be distinguished from Hanseniaspora occidentalis only by its maximum growth temperature.

In addition, we searched the genome for candidate genes underlying the physiological traits used for traditional identification in order to understand the genetic causes of yeasts metabolic diversity [20,82]. We analyzed the genome content of H. gamundiae and the publically available Hanseniaspora’s genomes for the presence of genes required for the utilization of disaccharides, as well as raffinose and glucono δ-lactone (Fig 4). As species of Hanseniaspora can assimilate only a limited number of carbon sources, they also mostly lack homologs of the genes required for their utilization. This fact partly explains the low number of ORFs in the genome of H. valbyensis predicted by Riley et al. [82] in a comparative study of yeasts belonging to subphylum Saccharomycotina. The only exception is presence of homologs of genes encoding predicted acid trehalase (ATH1) and neutral trehalase (NTH1), which are required for utilization of extracellular trehalose [83], a sugar on which none of the analyzed Hanseniaspora species can grow. Since these genes are also involved in the metabolism of trehalose manufactured inside the cell, it is possible that these genes play a role in the stress response or non-catabolic processes, instead.

Fig 4. Metabolic traits and genes for the assimilation of the carbon sources sucrose, raffinose, melibiose, galactose, lactose, trehalose, maltose, cellobiose, and glucono δ-lactone by Hanseniaspora species and Saccharomyce cerevisiae (S288c).

Numbered boxes indicate presence (1) or absence (0) of putative homologous genes determined by Reciprocal Best Hit (RBH) prediction algorithm. Physiological characteristics are from Kurtzman et al. [84], except for H. gamundiae.

One of the few sugars that H. gamundiae can assimilate and weakly ferment is sucrose, and this ability is strain-specific in its close relatives H. vineae and H. osmophila [84]. Unfortunately, no phenotypic data exists for H. vineae T02-19AF and H. osmophila AWRI 3579, the strains whose genome sequences are available [60,61]. Nevertheless, based on our genome sequence analyses (Fig 4), it seems likely that the presence of the SUC2 homolog encoding invertase is required for sucrose utilization in Hanseniaspora.

In contrast to the other Hanseniaspora species with available genomes, H. gamundiae is unable to assimilate glucono δ-lactone. In Saccharomyces cerevisiae, three enzymes are believed to be involved in metabolism of glucono δ-lactone [85] namely 6-phosphogluconolactonase encoded by SOL1 and SOL3, 6-phosphogluconate dehydrogenase encoded by GND1, and gluconokinase which might be encoded by the ORF YDR248C. We found that, even though it cannot consume the carbon source, H. gamundiae has homologs of all four genes that are thought to be essential for the growth on glucono δ-lactone. This discordance between phenotype and genotype in H. gamundiae is an additional example that metabolic traits of non-conventional yeasts cannot always be inferred from model organisms [20,86].

Morphologically both strains of H. gamundiae produced one to two sphaerical and warty ascospores (Fig 5), a feature shared with H. vineae and H. osmophila and not to its close relative of H. occidentalis. Strain CRUB 1604 is characterized by slow growth rate on standard yeast growth media (e.g. Yeast Malt Agar).

Fig 5. Hanseniapora gamundiae sp. nov. CRUB 1928T.

(a) Budding cells, YM broth, 25°C, 220 rpm, 2 days. (b) Sphaerical and warty ascospore, 5% malt extract agar after 21 days at 25°C. Scale bars, 10 μm.


Description of Hanseniaspora gamundiae Libkind, Čadež, Hittinger 2018, sp. nov. [Mycobank accession: MB824091].

Etymology: Specific epithet gamundiae (N.L. gen. fem. N.), “of Gamundi”, to honour Dr. Irma Gamundi (Argentina) in recognition for her valuable contributions on fungal systematics, particularly in the genus Cyttaria.

Standard description: The species belong to the genus Hanseniaspora in the Saccharomycetales. On YM agar, after 1 month at 25°C, the steak culture is cream colored, butyrous, smooth, glossy, and flat to slightly raised at the center, with an entire to slightly undulate margin. On slide culture with cornmeal agar, a rudimentary pseudomycelium is formed. In yeast extract-malt extract liquid medium after 48 h at 25°C, the cells are apiculate, ovoid, or elongate (4.3–15.7) μm × (2.4–4.7) μm; they occur singly or in pairs. Budding is bipolar. Sediment is present, and a very thin ring is formed after 1 month. Asci containing one to two sphaerical and warty ascospores (1.4–4.3 μm) are observed after 2 weeks or more on 5% malt extract agar and YM agar at 26°C. Ascospores are mostly not released from the ascus (Fig 2). Glucose and sucrose (weakly) are fermented; D-galactose, maltose, lactose, and cellobiose are not fermented. The carbon compounds that are assimilated are glucose, sucrose, cellobiose, salicin, and arbutin; no growth occurs on galactose, L-sorbose, D-glucosamine, N-acetyl-D-glucosamine, D-ribose, D-xylose, L-arabinose, D-arabinose, L-rhamnose, maltose, α,α-trehalose, methyl α-D-glucoside, melibiose, lactose, raffinose, melezitose, inulin, starch, glycerol, erythritol, ribitol, xylitol, L-arabinitol, D-glucitol, D-mannitol, galactitol, myo-inositol, glucono-δ-lactone, 2-keto-D-gluconate, D-gluconate, D-glucuronate, D-galacturonate, DL-lactate, succinate, citrate, methanol, ethanol, propane-1,2-diol, butane-2,3-diol, and hexadecane. Assimilation of nitrogen compounds is positive for ethylamine hydrochloride, lysine, and cadaverine, while it is negative for potassium nitrate, sodium nitrite, creatine, creatinine, glucosamine, and imidazole. Growth in vitamin-free medium is absent. Growth occurs at 30°C but is absent at 35°C. Growth with 10% NaCl is positive, but growth is absent with 16% NaCl, on 50% (w/w) glucose-yeast extract agar, with 1% acetic acid, and with 0.01% cycloheximide. The diazonium blue B reaction is negative. Unambiguous identification and phylogenetic placement is based on DNA sequences of the following nuclear loci: ITS/5.8S (KU674846), D1/D2 (KU674858), ACT1 (KU674870) and TEF1 (KU674882). The species habitats are Cyttaria hariotii stromata infecting Nothofagus spp. trees in Argentina.

The holotype CRUB 1928T was isolated from Cyttaria hariotii stromata infecting Nothofagus dombeyi “Coihue” collected at Perez Rosales pass, Patagonia, Argentina in spring 2007 and is preserved in a metabolically inactive state in the Centro Regional Universitario Bariloche Yeast Culture Collection, Argentina. Ex-type cultures are deposited at the Collection of Industrial Microorganisms, Slovenia (ZIM 2545T), ARS Culture Collection, National Center for Agricultural Utilization Research, IL, USA (NRRL Y-63793T), Portuguese Yeast Culture Collection, Portugal (PYCC 7262T) and at the University of Wisconsin-Madison, WI, USA (yHCT65T). The Mycobank number is MB824091. The BioProject number for raw genome sequencing reads is PRJNA434570 (BioSample SAMN08564278), and the GenBank accession number for the assembled genome is PTXO00000000.

A shift from phenotype- to sequence-based taxonomy enables introduction of the new International Code of Nomenclature for algae, fungi, and plants (Shenzhen Code; [22]) by which the teleomorphic genus Hanseniaspora has a priority over its anamorphic counterpart, Kloeckera, by the rules of nomenclature and the number of species assigned to each genus [23]. Accordingly, we propose the transfer of three Kloeckera species to the genus Hanseniaspora.

Description of Hanseniaspora hatyaiensis (Jindamorakot, Ninomiya, Limtong, Kawasaki & Nakase) Čadež & Libkind f.a., comb. nov. [MB 828569].

Basionym: Kloeckera hatyaiensis Jindamorakot, Ninomiya, Limtong, Kawasaki & Nakase (2009). FEMS Yeast Res 9: 1327–1337. [MB 514510]

Holotype ST-476; Ex-type cultures: BCC 14939, NBRC 104215, CBS 10842.

Description of Hanseniaspora lindneri (Klöcker) Čadež & Libkind f.a., comb. nov. [MB 828566].

Basionym: Pseudosaccharomyces lindneri Klöcker (1912). Zentralbl. Bakteriol. Parasitenkd., Abt. II, 35: 375–388. [MB 180162]

Kloeckera lindneri (Klöcker) Janke (1928). Zentralbl. Bakteriol. Parasitenkd., Abt. II, 76: 161. [MB 467907]

Holotype CBS 285; Ex-type culture: NRRL Y-17531.

Description of Hanseniaspora taiwanica (Lee) Čadež & Libkind f.a., comb. nov. [MB 828567].

Basionym: Kloeckera taiwanica C.F. Lee (2012), Int J Syst Evol Microbiol 62:1434–1437. [MB 561891]

Holotype EJ7M09; Ex-type cultures: BCRC 23182, CBS 11434.

Supporting information

S1 Table. List of the strains studied, their origins, and their GenBank accession numbers.


S2 Table. Similarities among closely related genomes.

The values are presented as the Alignment-Free Distance Measure (Kr), Average Nucleotide Identity (ANI) and by estimating digital DNA-DNA Homology values (dDDH values) in comparison to DNA-DNA reassociation [36,62] where available.


S1 Fig. UPGMA dendrogram based on PCR fingerprints obtained with the microsatellite primers (GTG)5x and (ATG)5x on Hanseniaspora gamundiae sp. nov. and their closest relatives.

The distances between the strains were computed using Pearson's correlation coefficient.



We thank Irene Ouoba for providing the type strain of Hanseniaspora jakobsenii, the Argentinean National Park Administration for sample collection permits, as well as Martin Bontrager and Amanda Beth Hulfachor for Illumina library preparation, Jacek Kominek and Quinn K. Langdon for data processing, and the University of Wisconsin Biotechnology Center DNA Sequencing Facility for providing Illumina sequencing facilities and services.


  1. 1. Čadež N, Raspor P, Smith MT. Phylogenetic placement of Hanseniaspora-Kloeckera species using multigene sequence analysis with taxonomic implications: descriptions of Hanseniaspora pseudoguilliermondii sp. nov. and Hanseniaspora occidentalis var. citrica var. nov. Int J Syst Evol Microbiol. 2006;56: 1157–1165. pmid:16627671
  2. 2. Čadež N, Pagnocca FC, Raspor P, Rosa CA. Hanseniaspora nectarophila sp nov., a yeast species isolated from ephemeral flowers. Int J Syst Evol Microbiol. 2014;64: 2364–2369. pmid:24763602
  3. 3. Jindamorakot S, Ninomiya S, Limtong S, Yongmanitchai W, Tuntirungkij M, Potacharoen W, et al. Three new species of bipolar budding yeasts of the genus Hanseniaspora and its anamorph Kloeckera isolated in Thailand. FEMS Yeast Res. 2009;9: 1327–1337. pmid:19788563
  4. 4. Chang CF, Huang LY, Chen SF, Lee CF. Kloeckera taiwanica sp. nov., an ascomycetous apiculate yeast species isolated from mushroom fruiting bodies. Int J Syst Evol Microbiol. 2012;62: 1434–1437. pmid:21841004
  5. 5. Ouoba LII, Nielsen DS, Anyogu A, Kando C, Diawara B, Jespersen L, et al. Hanseniaspora jakobsenii sp nov., a yeast isolated from Bandji, a traditional palm wine of Borassus akeassii. Int J Syst Evol Microbiol. 2015;65: 3576–3576 pmid:26297247
  6. 6. Groenewald M, Lombard L, de Vries M, Giraldo Lopez M, Smith M, Crous PW. Diversity of yeast species from Dutch garden soil and the description of six novel Ascomycetes, FEMS Yeast Research, 2018;18(7): Forthcoming.
  7. 7. Kurtzman CP, Mateo RQ, Kolecka A, Theelen B, Robert V, Boekhout T. Advances in yeast systematics and phylogeny and their use as predictors of biotechnologically important metabolic pathways. FEMS Yeast Res. 2015;15. pii: fov050. pmid:26136514
  8. 8. Daniel HM, Sorrell TC, Meyer W. Partial sequence analysis of the actin gene and its potential for studying the phylogeny of Candida species and their teleomorphs. Int J Syst Evol Microbiol. 2001;51: 1593–1606. pmid:11491363
  9. 9. Kurtzman CP, Robnett CJ. Phylogenetic relationships among yeasts of the 'Saccharomyces complex' determined from multigene sequence analyses. FEMS Yeast Res. 2003;3: 417–32. pmid:12748053
  10. 10. Kurtzman CP, Robnett CJ. Relationships among genera of the Saccharomycotina (Ascomycota) from multigene phylogenetic analysis of type species. FEMS Yeast Res.2013;13: 23–33. pmid:22978764
  11. 11. Rokas A, Williams BL, King N, Carroll SB. Genome-scale approaches to resolving incongruence in molecular phylogenies. Nature. 2003;425:798–804. pmid:14574403
  12. 12. Fitzpatrick DA, Logue ME, Stajich JE, Butler G. A fungal phylogeny based on 42 complete genomes derived from supertree and combined gene analysis. BMC Evol Biol. 2006;6.
  13. 13. Shen XX, Zhou X, Kominek J, Kurtzman CP, Hittinger CT, Rokas A. Reconstructing the backbone of the Saccharomycotina yeast phylogeny using genome-scale data. G3 (Bethesda). 2016;6: 3927–3939.
  14. 14. Kuramae EE, Robert V, Snel B, Weiss M, Boekhout T. Phylogenomics reveal a robust fungal tree of life. FEMS Yeast Res.2006;6: 1213–1220. pmid:17156018
  15. 15. Varghese NJ, Mukherjee S, Ivanova N, Konstantinidis KT, Mavrommatis K, Kyrpides NC, et al. Microbial species delineation using whole genome sequences. Nucleic Acids Res. 2015;43: 6761–6771. pmid:26150420
  16. 16. Libkind D, Hittinger CT, Valério E, Gonçalves C, Dover J, Johnston M, et al. Microbe domestication and the identification of the wild genetic stock of lager-brewing yeast. Proc Natl Acad Sci USA. 2011;108: 14539–44. pmid:21873232
  17. 17. Dietrich FS, Voegeli S, Kuo S, Philippsen P. Genomes of Ashbya fungi isolated from insects reveal four mating-type loci, numerous translocations, lack of transposons, and distinct gene duplications. G3 (Bethesda). 2013;3: 1225–1239.
  18. 18. Hittinger CT, Rokas A, Bai FY, Boekhout T, Goncalves P, Jeffries TW, et al. Genomics and the making of yeast biodiversity. Curr Opin Genetics Dev. 2015;35: 100–109.
  19. 19. Lopes MR, Morais CG, Kominek J, Cadete RM, Soares MA, Uetanabaro AP, et al. Genomic analysis and D-xylose fermentation of three novel Spathaspora species: Spathaspora girioi sp. nov., Spathaspora hagerdaliae f. a., sp. nov. and Spathaspora gorwiae f. a., sp. nov. FEMS Yeast Res. 2016;16(4).
  20. 20. Haase MAB, Kominek J, Langdon QK, Kurtzman CP, Hittinger CT. Genome sequence and physiological analysis of Yamadazyma laniorum f.a. sp. nov. and a reevaluation of the apocryphal xylose fermentation of its sister species Candida tenuis. FEMS Yeast Res. 2017: 1;17(3). pmid:28419220
  21. 21. Lee DK, Hsiang T, Lachance MA. Antonie Leeuwenhoek. Metschnikowia mating genomics. 2018.
  22. 22. Turland NJ, Wiersema JH, Barrie FR, Greuter W, Hawksworth DL, Herendeen PS, Knapp S, Kusber W-H, Li D-Z, Marhold K, May TW, McNeill J, Monro A M, Prado J, Price MJ, Smith GF, editors. International Code of Nomenclature for algae, fungi, and plants (Shenzhen Code) adopted by the Nineteenth International Botanical Congress Shenzhen, China, July 2017. Regnum Vegetabile 159. Glashütten: Koeltz Botanical Books. 2018.
  23. 23. Daniel HM, Lachance MA, Kurtzman CP. On the reclassification of species assigned to Candida and other anamorphic ascomycetous yeast genera based on phylogenetic circumscription. Antonie Leeuwenhoek. 2014;106: 67–84. pmid:24748333
  24. 24. Péter G, Takashima M, Čadež N. Yeast Habitats: Different but Global. In: Buzzini P, Lachance M-A, Yurkov A, editors. Yeasts in Natural Ecosystems: Ecology. Cham: Springer; 2017. pp. 39–71.
  25. 25. Lam SS, Howell KS (2015) Drosophila-associated yeast species in vineyard ecosystems. FEMS Microbiol Lett 362:fnv170. pmid:26391524
  26. 26. Abranches J, Starmer WT, Hagler AN. Yeast-yeast interactions in guava and tomato fruits. Microb Ecol. 2001;42: 186–192. pmid:12024281
  27. 27. Libkind D, Ruffini A, van Broock M, Alves L, Sampaio JP. Biogeography, host specificity, and molecular phylogeny of the basidiomycetous yeast Phaffia rhodozyma and its sexual form, Xanthophyllomyces dendrorhous. Appl Environ Microbiol. 2007;73: 1120–1125. pmid:17189439
  28. 28. Ulloa JA, Libkind D, Fontenla SB, van Broock M. Levaduras fermentadoras aisladas de Cyttaria hariotii (Fungi) en bosques Andino-Patagonicos (Argentina). Bol Soc Argent Bot. 2009;44: 239–248.
  29. 29. Buzzini P, Lachance M-A, Yurkov A, editors. Yeasts in Natural Ecosystems: Diversity. Cham: Springer; 2017.
  30. 30. Khan IA, Abourashed EA. Leung’s encyclopedia of common natural ingredients. 3rd ed. Hoboken, New Jersey: John Wiley & Sons, Inc.; 2010.
  31. 31. Phaff HJ. Hanseniaspora Zikes. In: Lodder J, editor. The Yeasts, A Taxonomic Study. 2nd ed. Amsterdam: North-Holland; 1970. pp. 209–225.
  32. 32. Almeida P, Barbosa R, Zalar P, Imanishi Y, Shimizu K, Turchetti B, et al. A population genomics insight into the Mediterranean origins of wine yeast domestication. Mol Ecol. 2015;24: 5412–5427. pmid:26248006
  33. 33. Eizaguirre JI, Peris D, Rodríguez ME., Lopes CA, De Los Ríos P, Hittinger CT, Libkind D. Phylogeography of the wild Lager-brewing ancestor (Saccharomyces eubayanus) in Patagonia. Environ Microbiol. 2018;20:3732–3743. pmid:30105823
  34. 34. Sampaio JP, Goncalves P. Natural populations of Saccharomyces kudriavzevii in Portugal are associated with oak bark and are sympatric with S. cerevisiae and S. paradoxus. Appl Environ Microbiol. 2008;74: 2144–2152. pmid:18281431
  35. 35. Kurtzman CP, Fell JW, Boekhout T. Methods for isolation, phenotypic characterization and maintenance of yeasts. In: Kurtzman CP, Fell JW, Boekhout T, editors. The Yeasts, a Taxonomic Study. 5 ed. Amsterdam: Elsevier; 2011. pp. 87–110.
  36. 36. Cadez N, Poot GA, Raspor P, Smith MT. Hanseniaspora meyeri sp. nov., Hanseniaspora clermontiae sp. nov., Hanseniaspora lachancei sp. nov and Hanseniaspora opuntiae sp. nov., novel apiculate yeast species. Int J Syst Evol Micr. 2003;53: 1671–1680.
  37. 37. Edgar RC. MUSCLE: multiple sequence alignment with high accuracy and high throughput, Nucleic Acids Res. 2004;32: 1792–97. pmid:15034147
  38. 38. Tamura K, Nei M. Estimation of the number of nucleotide substitutions in the control region of mitochondrial-DNA in humans and chimpanzees. Mol Biol Evol. 1993;10: 512–526. pmid:8336541
  39. 39. Tamura K, Stecher G, Peterson D, Filipski A, Kumar S. MEGA6: Molecular evolutionary genetics analysis version 6.0. Mol Biol Evol. 2013;30: 2725–2729. pmid:24132122
  40. 40. Felsenstein J. Confidence-limits on phylogenies—an approach using the bootstrap. Evolution. 1985;39: 783–791. pmid:28561359
  41. 41. Huson D.H. and Bryant D., Application of Phylogenetic Networks in Evolutionary Studies, Molecular Biology and Evolution, 23(2):254–267, 2006. pmid:16221896
  42. 42. Clement M, Posada D, Crandall KA. TCS: a computer program to estimate gene genealogies. Mol Ecol. 2000;9: 1657–1659. pmid:11050560
  43. 43. Cadez N, Raspor P, de Cock AW, Boekhout T, Smith MT. Molecular identification and genetic diversity within species of the genera Hanseniaspora and Kloeckera. FEMS Yeast Res. 2002;1: 279–289. pmid:12702331
  44. 44. Bellora N, Moline M, David-Palma M, Coelho MA, Hittinger CT, Sampaio JP, et al. Comparative genomics provides new insights into the diversity, physiology, and sexuality of the only industrially exploited tremellomycete: Phaffia rhodozyma. BMC Genomics. 2016;17: 901. pmid:27829365
  45. 45. Hittinger CT, Goncalves P, Sampaio JP, Dover J, Johnston M, Rokas A. Remarkably ancient balanced polymorphisms in a multi-locus gene network. Nature. 2010;464: 54–58. Epub 2010/02/19. pmid:20164837
  46. 46. Bankevich A, Nurk S, Antipov D, Gurevich AA, Dvorkin M, Kulikov AS, et al. SPAdes: a new genome assembly algorithm and its applications to single-cell sequencing. J Comp Biol. 2012;19: 455–477.
  47. 47. Kent WJ. BLAT—the BLAST-like alignment tool. Genome Res. 2002;12: 656–664. pmid:11932250
  48. 48. Smit A, Hubley R, Green P. RepeatMasker Open-3.0. 1996–2010; Available from:
  49. 49. Jurka J, Kapitonov VV, Pavlicek A, Klonowski P, Kohany O, Walichiewicz J. RepBase Update, a database of eukaryotic repetitive elements. Cytogenet Genome Res. 2005;110: 462–467. pmid:16093699
  50. 50. Lowe TM, Eddy SR. tRNAscan-SE: a program for improved detection of transfer RNA genes in genomic sequence. Nucleic Acids Res. 1997;25: 955–964. pmid:9023104
  51. 51. Ter-Hovhannisyan V, Lomsadze A, Chernoff YO, Borodovsky M. Gene prediction in novel fungal genomes using an ab initio algorithm with unsupervised training. Genome Res. 2008;18: 1979–1990. pmid:18757608
  52. 52. Engel SR, Dietrich FS, Fisk DG, Binkley G, Balakrishnan R, Costanzo MC, et al. The reference genome sequence of Saccharomyces cerevisiae: then and now. G3 (Bethesda). 2014;4: 389–398.
  53. 53. Conesa A, Gotz S, Garcia-Gomez JM, Terol J, Talon M, Robles M. Blast2GO: a universal tool for annotation, visualization and analysis in functional genomics research. Bioinformatics. 2005;21: 3674–3676. pmid:16081474
  54. 54. Gremme G, Steinbiss S, Kurtz S. GenomeTools: A comprehensive software library for efficient processing of structured genome annotations. IEEE ACM T Comput Bi. 2013;10: 645–656.
  55. 55. Yoon SH, Ha SM., Lim JM, Kwon SJ, Chun J. A large-scale evaluation of algorithms to calculate average nucleotide identity. Antonie Leeuwenhoek. 2017;110:1281–1286. pmid:28204908
  56. 56. Meier-Kolthoff JP, Auch AF, Klenk HP, Goker M. Genome sequence-based species delimitation with confidence intervals and improved distance functions. BMC Bioinformatics. 2013;14. pmid:23432962
  57. 57. Kurtzman CP, Robnett CJ. Identification and phylogeny of ascomycetous yeasts from analysis of nuclear large subunit (26S) ribosomal DNA partial sequences. Antonie Leeuwenhoek. 1998;73: 331–371. pmid:9850420
  58. 58. Lachance MA, Wijayanayaka TM, Bundus JD, Wijayanayaka DN. Ribosomal DNA sequence polymorphism and the delineation of two ascosporic yeast species: Metschnikowia agaves and Starmerella bombicola. FEMS Yeast Res. 2011;11:324–333. pmid:21251208
  59. 59. Yurkov A, Guerreiro MA, Sharma L, Carvalho C, Fonseca Á (2015) Correction: Multigene Assessment of the Species Boundaries and Sexual Status of the Basidiomycetous Yeasts Cryptococcus flavescens and C. terrestris (Tremellales). PLOS ONE 10(4): e0126996. pmid:25910228
  60. 60. Giorello FM, Berna L, Greif G, Camesasca L, Salzman V, Medina K, et al. Genome sequence of the native apiculate wine yeast Hanseniaspora vineae T02/19AF. Genome Announc. 2014;2. Epub 2014/05/31.
  61. 61. Sternes PR, Lee D, Kutyna DR, Borneman AR. Genome sequences of three species of Hanseniaspora isolated from spontaneous wine fermentations. Genome Announc. 2016;4. Epub 2016/11/20.
  62. 62. Meyer SA, Smith MT, Simione FP. Systematics of Hanseniaspora Zikes and Kloeckera Janke. Antonie Leeuwenhoek. 1978;44: 79–96. pmid:566079
  63. 63. Wicker T, Sabot F, Hua-Van A, Bennetzen JL, Capy P, Chalhoub B, et al. A unified classification system for eukaryotic transposable elements. Nat Rev Genet. 2007;8: 73–82.
  64. 64. Bleykasten-Grosshans C, Neuveglise C. Transposable elements in yeasts. Cr Biol. 2011;334: 679–86.
  65. 65. Parra G, Bradnam K, Ning Z, Keane T, Korf I. Assessing the gene space in draft genomes. Nucleic Acids Res. 2009;37: 289–297. pmid:19042974
  66. 66. Kalač P. A review of chemical composition and nutritional value of wild-growing and cultivated mushrooms. J Sci Food Agr. 2013;93: 209–218.
  67. 67. Yurkov A,. Pozo M. Yeast Community Composition and Structure. In: Buzzini P, Lachance M-A, Yurkov A, editors. Yeasts in Natural Ecosystems: Ecology. Cham: Springer; 2017. pp. 73–100.
  68. 68. De Lederkremer RM, Cirelli A. Hidratos de carbono en hongos del género Cyttaria. Su importancia. Anales Acad Ci Exact Natur 1988;4: 153–61.
  69. 69. Gamundí IJ, De Lederkremer RM. Los Hongos Andino-Patagónicos del género Cyttaria. Sus hidratos de carbono. Ciencia e Investigación. 1989;43: 4–13.
  70. 70. Pardo LO, Pizarro JL. La chicha en el Chile Precolombino. Santiago: Editorial Mare Nostrum; 2005.
  71. 71. Mösbach EW. Botanica indigena de Chile. In: Aldunate C, Villagran C, editors. Museo Chileno de Arte Precolombino. Santiago de Chile: Fundación Andes y Editorial Andrés Bello; 1991.
  72. 72. Fátima CO, Inayara G, Lacerda CA, Libkind D, Lopes CA, Carvajal J, Rosa CA. Traditional foods and beverages from South America: microbial communities and production strategies. In: Krause J, Fleischer O, editors. Industrial Fermentation: Food Processes, Nutrient Sources; and Production Strategies. New York: Nova Science Publishers; 2010. pp. 79–114.
  73. 73. Wang C, Mas A, Esteve-Zarzoso B. Interaction between Hanseniaspora uvarum and Saccharomyces cerevisiae during alcoholic fermentation. Int J Food Microbiol, 2015;206: 67–74. pmid:25956738
  74. 74. Lleixà J, Martín V, Portillo MC, Carrau F, Beltran G, Mas A. Comparison of fermentation and wines produced by inoculation of Hanseniaspora vineae and Saccharomyces cerevisiae. Front Microbiol. 2016;7: 338. pmid:27014252
  75. 75. Dott W, Heinzel M, Trüper HG. Sulfite formation by wine yeasts. I. Relationships between growth, fermentation and sulfite formation. Arch Microbiol. 1976;107: 289–292.
  76. 76. Rauhut D. Usage and formation of sulphur compounds. In: König H, Unden G, Fröhlich J, editors. Biology of Microorganisms on Grapes, in Must and in Wine. Berlin Heidelberg: Springer-Verlag; 2009. pp. 181–207.
  77. 77. Grant CM, MacIver FH, Dawes IW. Glutathione is an essential metabolite required for resistance to oxidative stress in the yeast Saccharomyces cerevisiae. Curr. Genet. 1996;29: 511–515. pmid:8662189
  78. 78. Odat O, Matta S, Khalil H, Kampranis SC, Pfau R, Tsichlis PN, Makris AM. Old yellow enzymes, highly homologous FMN oxidoreductases with modulating roles in oxidative stress and programmed cell death in yeast. J Biol Chem. 2007; 282: 36010–23. pmid:17897954
  79. 79. Felder T, Bogengruber E, Tenreiro S, Ellinger A, Sá-Correia I, Briza P. Dtr 1p, a multidrug resistance transporter of the major facilitator superfamily, plays an essential role in spore wall maturation in Saccharomyces cerevisiae. Eukaryot Cell. 2002;1: 799–810. pmid:12455697
  80. 80. Gbelska Y, Krijger JJ, Breunig KD. Evolution of gene families: the multidrug resistance transporter genes in five related yeast species. FEMS Yeast Res. 2006;6: 345–55. pmid:16630275
  81. 81. Almeida P, Barbosa R, Bensasson D, Gonçalves P, Sampaio JP. Adaptive divergence in wine yeasts and their wild relatives suggests a prominent role for introgressions and rapid evolution at noncoding sites. Mol Ecol. 2017;26: 2167–2182. pmid:28231394
  82. 82. Riley R, Haridas S, Wolfe KH, Lopes MR, Hittinger CT, Göker M, et al. Comparative genomics of biotechnologically important yeasts. Proc Natl Acad Sci USA, 2016;113: 9882–87. pmid:27535936
  83. 83. Jules M, Guillou V, Franǫis J, Parrou J-L. Two distinct pathways for trehalose assimilation in the yeast Saccharomyces cerevisiae. Appl Environ Microbiol. 2004;70: 2771–2778. pmid:15128531
  84. 84. Kurtzman CP, Fell JW, Boekhout T, The Yeasts, a Taxonomic Study. 5 ed. Amsterdam: Elsevier; 2011.
  85. 85. Sinha A, Maitra PK. Induction of specific enzymes of the oxidative pentose phosphate pathway by glucono-delta-lactone in Saccharomyces cerevisiae. J Gen Microbiol. 1992;138: 1865–73. 76. pmid:1328471
  86. 86. Opulente DA, Rollinson EJ, Bernick-Roehr C, Hulfachor AB, Rokas A, Kurtzman CP, et al. Factors driving metabolic diversity in the budding yeast subphylum. BMC Biology. 2018;16(1):26. pmid:29499717