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A novel aminotransferase gene and its regulator acquired in Saccharomyces by a horizontal gene transfer event



Horizontal gene transfer (HGT) is an evolutionary mechanism of adaptive importance, which has been deeply studied in wine S. cerevisiae strains, where those acquired genes conferred improved traits related to both transport and metabolism of the nutrients present in the grape must. However, little is known about HGT events that occurred in wild Saccharomyces yeasts and how they determine their phenotypes.


Through a comparative genomic approach among Saccharomyces species, we detected a subtelomeric segment present in the S. uvarum, S. kudriavzevii, and S. eubayanus species, belonging to the first species to diverge in the Saccharomyces genus, but absent in the other Saccharomyces species. The segment contains three genes, two of which were characterized, named DGD1 and DGD2. DGD1 encodes dialkylglicine decarboxylase, whose specific substrate is the non-proteinogenic amino acid 2-aminoisobutyric acid (AIB), a rare amino acid present in some antimicrobial peptides of fungal origin. DGD2 encodes putative zinc finger transcription factor, which is essential to induce the AIB-dependent expression of DGD1. Phylogenetic analysis showed that DGD1 and DGD2 are closely related to two adjacent genes present in Zygosaccharomyces.


The presented results show evidence of an early HGT event conferring new traits to the ancestor of the Saccharomyces genus that could be lost in the evolutionary more recent Saccharomyces species, perhaps due to loss of function during the colonization of new habitats.


Yeasts of the Saccharomyces genus have been used for different industrial processes such as winemaking, brewing, and bakery. Many studies have aimed to dissect the molecular foundations that underline the traits of biotechnological interest such as those related to nutrient consumption. Among the mechanisms responsible for the acquisition of new functions, the horizontal (or lateral) gene transfer (HGT or LGT) has gained more attention as an important evolutionary process involved in fungi and yeast adaptation to specific environments [1]. HGT is the acquisition from a distantly related species of xenologous genes, which provide either improved or novel biological functions that might confer a competitive advantage during environmental selective pressures [2].

In recent years, the vast availability of genome sequences of different yeast species and strains allowed the identification of more genes likely acquired through HGT [3, 4]. They are normally detected through phylogeny inference, where the topology of a candidate gene contradicts the established species’ phylogeny [1, 2]. In S. cerevisiae, most reported HGT events encode putative proteins related to metabolic processes such as the metabolism and transport of carbon and nitrogen sources [3, 5]. However, few studies have experimentally validated their function and physiological role. A well-reported prokaryote-to-eukaryote gene transfer in S. cerevisiae is the gene URA1, encoding a dihydroorotate dehydrogenase, which was acquired from a lactic acid bacterium to allow the anaerobic biosynthesis of orotate. It is believed this was an important evolutionary step for the adaption of S. cerevisiae to anaerobic environments [5]. In addition, eukaryote-to-eukaryote gene transfers have also been described in wine S. cerevisiae isolates which conferred an important advantage to growth in fermentative environments. In particular, the large genomic segments named regions B and C were acquired from Zygosaccharomyces bailii and Torulaspora microellipsoides, respectively [3, 6]. Region C contains the FOT1-2 genes, encoding oligopeptide permeases, and the gene FSY1, codifying for a high-affinity fructose/H + symporter, which conferred the ability to uptake oligopeptides and the high fructose amounts present in the grape must, respectively [6, 7]. Nevertheless, there is still little experimental evidence about which HGT events have occurred in natural niches among wild Saccharomyces isolates.

Through a genomic comparative approach, we found a small 7-kb subtelomeric segment, containing three putative genes related to nitrogen metabolism, present in the species S. uvarum, S. kudriavzevii, and S. eubayanus, but absent in the remaining Saccharomyces species. In the present study, we report the characterization of two of these genes, one named DGD1 encoding a yeast dialkylglycine decarboxylase, and the second DGD2 codifying its putative regulator.

Dialkylglycine decarboxylase (DGDA) has first been described in the bacterium Burkholderia cepacia [8], and later in some fungi [9, 10]. This enzyme belongs to the aminotransferase class III, which uses either α-ketoglutarate or pyruvate as the preferred amino group acceptors, and the pyridoxal phosphate (PLP) as a cofactor, that covalently binds to the amino group of their substrates, which is normally located at end of the alkyl chain and generally distal to the carboxylate group. However, DGDA is one of the few exceptions to this aminotransferase family that binds to the alpha-amino group [11]. The enzyme exhibits the unique ability to catabolize the non-proteogenic dialkylamino acid 2-aminoisobutyric acid (AIB), which is present in soils and is an important component of the fungal antimicrobial oligopeptides called peptaibols [8, 12]. DGDA catalyzes AIB through two half-reactions (Fig. 1): (1) The AIB binds to the PLP pyridoxal ring to form an external aldimine followed by a decarboxylation reaction (first half-reaction) which releases CO2. (2) Then the formed quinonoid intermediate is reduced to form pyridoxamine phosphate (PMP) and an acetone molecule is released. (3) The PMP suffers a transamination reaction (second half-reaction) in which its amino group is transferred to a pyruvate molecule to form alanine and recycle the PLP [13].

Fig. 1
figure 1

Dialkylglycine decarboxylase reaction. The aminotransferase catalyzes the AIB through two half-reactions. The first step corresponds to AIB decarboxylation releasing CO2. The second, to the transamination of the amino group of the intermediate PMP to the pyruvate that produces L-alanine [13, 14]

In addition, we also identified a putative regulator of DGD1, named DGD2, that contains the characteristic functional motif of the zinc binuclear proteins. These proteins are known to be exclusive to fungi and are involved in the regulation of various physiological processes such as the induction of genes necessary for the metabolism of specific amino acids, for example, the well-reported regulator proteins Cha4p, Aro80p, and Leu3p, among others [15, 16].

Phylogenetic analysis showed that genes DGD1 and DGD2 might have been acquired by HGT from a member of the Zygosaccharomyces genus. The findings and experimental validation of this study show for the first time the evidence of an HGT event in non-S. cerevisiae species are involved in their adaptation to natural environments, in which dialkyl amino acid-containing peptaibols are released by fungi during microbial warfare.


Identification of a yeast dialkylglycine decarboxylase-like gene

Reannotations of the genomes of S. uvarum CBS7001 and S. kudriavzevii IFO1802 revealed a novel cluster composed of three genes with unknown functions. This cluster is conserved between both S. uvarum and S. kudriavzevii genomes and is absent in the S. cerevisiae reference strain S288C. The blastx search of these three genes against the non-redundant protein sequence database revealed the presence of this cluster in other strains of S. uvarum and S. kudriavzevii, and in an additional Saccharomyces species, S. eubayanus. The absence of this cluster in the rest of the Saccharomyces species was confirmed using the blastn algorithm against both the non-redundant database and Saccharomyces genome assemblies (Additional file 1: Table S1). The blastn search showed that the three genes may encode a putative zinc finger transcription factor (TF) similar to that encoded by the gene CHA4, an Aminotransferase-like protein (AT), and a putative amino acid permease (AAP). We obtain the deduced amino acid sequences from the AT-encoding genes of the Saccharomyces strains. The consensus sequence was used to define possible protein domains according to the PROSITE database. The analysis showed that AT contains a pyridoxal phosphate (PLP)-attachment site (Fig. 2) which belongs to the aminotransferase class III family [11]. The Blastp search of the predicted amino acid consensus sequence against the Swissprot database and a subsequent CLUSTAL Omega alignment showed that the AT shares 51.9% of identity with the Burkholderia cepacia dialkylglicine decarboxylase (DGDA) enzyme, whose substrate is the non-proteinogenic amino acid 2-aminoisobutyric acid (AIB) [8]. Moreover, the reported residues (Q52, W138, M141, S215, K272, and R406) to be involved at the subsites (A, B, and C) of the B. cepacia DGDA active site [14] are conserved in the yeast AT protein sequence (Fig. 2). Thus, this data suggests that the gene AT, hereafter referred to as DGD1, may encode a dialkylglicine decarboxylase enzyme, and those yeast strains carrying the gene DGD1 could display a dialkylglycine carboxylase activity.

Fig. 2
figure 2

Dialkylglycine decarboxylase active site. The alignment between Saccharomyces AT and B. cepacia DGDA sequences shows that the PLP-binding domain (obtained from the PROSITE database) and residues involved in the catabolism of AIB are conserved in the deduced AT amino acid sequence. The scheme was adapted from [13, 14]

Saccharomyces isolates with DGD1 can use 2-aminoisobutyric acid as a nitrogen source

Since it has been reported that E. coli expressing the B. cepacia DGDA gene acquired the ability to metabolize AIB [8] and S. cerevisiae is unable to use AIB nitrogen sources [17], we tested the ability of the Saccharomyces isolates carrying the gene DGD1 (S. eubayanus, S. uvarum, and S. kudriavzevii) to use AIB as the sole nitrogen source. Therefore, we took different strains belonging to the species S. eubayanus, S. uvarum, S. kudriavzevii, and S. cerevisiae (Table 1) and plated them on YNB solid media at different AIB concentrations (1 mM, 5 mM, and 10 mM). After 11 days, the S. kudriavzevii strains IFO1802 and CR85 and, to a lesser extent, CR90 and CBS12751, were able to grow in the presence of AIB, and at major concentrations, a better growth was observed especially in the strain IFO1802 (Fig. 3, third column). The S. uvarum strains BMV58 and CBS7001 grew very poorly, but better than NPCC1290 and NPCC1314 (Fig. 3). However, none of the S. eubayanus strains were able to grow in these conditions. As expected, no growth was observed in the S. cerevisiae strains and all the Saccharomyces isolates exhibited optimal growth in the presence of glutamine after 4 days (Fig. 3, fourth column). These results demonstrated that some Saccharomyces isolates carrying the gene DGD1 can grow in the presence of AIB, with variable growth rates depending on the species and strain. These results suggested that the novel DGD1 gene may be responsible for the use of AIB as a nitrogen source.

Table 1 Wild and reference strains used in this study
Fig. 3
figure 3

Growth screening of Saccharomyces isolates. The strains were cultured on YNB plates at the different AIB concentrations and 10 mM Glutamine (Gln) as the sole nitrogen source

DGD1 confers the ability to use AIB as a nitrogen source

To test whether the gene DGD1 is responsible for the dialkylglycine decarboxylase activity or not, we generated mutant strains of the entire cluster and mutants of each gene in both BMV58 and IFO1802 backgrounds, which respectively showed the best phenotypes among the tested S. uvarum and S. kudriavzevii isolates (Fig. 3). Moreover, the S. kudriavzevii IFO1802 strain contains two copies of these subtelomeric genes, located at chromosomes VII and X. The latter carries DGD1 and APP alleles containing one indel that completely changes the reading frame and produces premature stop codons (Fig. 4). Once we generated the mutant strains (Table 2), they were cultured on YNB 10 mM AIB plates. Due to the slow growth rate exhibited by the S. uvarum strain BMV58 in the tested conditions, we also assayed the resistance against the growth inhibitory effect exerted by AIB [17]. We cultured the cells in the presence of AIB with either 10 mM glutamine or 10 mM proline. Additionally, we used either 10 mM glutamine or 10 mM proline as the sole nitrogen source as a control medium (Fig. 4). Glutamine, as a preferred nitrogen source, activates the nitrogen catabolite repression (NCR), a wide transcriptional regulation program enabling Saccharomyces yeast to repress genes involved in the utilization of poor and rare nitrogen sources when preferred ones are available. However, proline, as a poor nitrogen source, does not activate NCR. Among the repressed genes by NCR is GAP1, encoding a general amino acid permease involved in the uptake of all L-amino acids, some D-amino acids, related compounds, toxic analogs, and polyamines, likely including AIB.

Fig. 4
figure 4

Growth and resistance against AIB phenotypes of the mutant strains. Above, the chromosome localization of the subtelomeric genes and the applied gene disruption approach to both strains IFO1802 and AQ2901 are shown. Below, the ability to use AIB as the sole nitrogen source (column AIB) and the resistance against the AIB’s inhibitory growth effect (columns P, AIB + P, G & AIB + G) exhibited by parental and mutant strains are depicted. G: 10 mM glutamine; P: 10 mM proline; AIB: 10 mM 2-aminoisobutyric acid

Table 2 Engineered strains used in this study

As we demonstrated above, the haploid S. uvarum BMV58-derived strain AQ2901 grew also after 11 days in the presence of AIB as the sole nitrogen source (Fig. 4, AIB column). However, the deletant strains Su-ClusterΔ and Su-DGD1Δ were unable to grow in this condition (Fig. 4, AIB column). Additionally, these strains showed decreased resistance against AIB after 4 days (Fig. 4, AIB + P column). But in the presence of glutamine, the inhibitory effect was negligible (Fig. 4, AIB + G column). As we expected, all the strains showed optimal growth on glutamine and proline as sole nitrogen sources (Fig. 4, P & G columns). We observed similar effects in the IFO1802 deletants Sk-ClusterΔ and Sk-DGD1Δ, which did not grow in the presence of AIB after 4 days (Fig. 4, AIB column). Additionally, the resistance against AIB was lost and hence no growth was observed in both mutants (Fig. 4, column AIB + P). Both Su-AAP∆ and Sk-AAP∆ mutants showed the same growth phenotype as their parental strains (Fig. 4). Surprisingly, the strains Su-TF and Sk-TF, which are mutants in the TF gene that encodes a putative Zing-finger transcription factor, showed similar phenotypes as the mutants Su-DGD1 and Sk-DGD1. Interestingly, the strain Sk-TF showed a little residual growth (Fig. 4, column AIB + P). These results suggest that gene DGD1 might encode a dialkylglicine decarboxylase enzyme and the gene TF, from now named DGD2, could be involved in the regulation of the dialkylglycine activity.

DGD1 encodes a yeast dialkylglycine decarboxylase enzyme

To confirm the gene DGD1 encodes a dialkylglycine decarboxylase enzyme, we cloned both S. kudriavzevii IFO1802 and S. uvarum AQ2901 DGD1 genes (Additional files 2, 3, 4 and 5: Figs. S1-S4, respectively) into the expression plasmid pYES2.1 TOPO® TA to construct the plasmids pYES-Sk-DGD1 and pYES-Su-DGD1 (Table 4). They were used to transform the host S. cerevisiae lab yeast CML235 to generate the strains CML235-DGD1-Sk and CML235-DGD1-Su, respectively (Table 2). When both yeasts were cultured in a minimal medium with AIB (Fig. 5A), they showed an increment of about 30–40% of the µmax compared to the control strain CML235-LacZ. We also assayed the protein production kinetics by Western blot and observed a high protein production after 3 h of growth in the inducer medium, which was maintained constant until 24 h in the strains CML235-DGD1-Sk and CML235-DGD1-Su and 12 h for CML235-LacZ (Fig. 5B). Then, we quantified the transformation of AIB to acetone, the by-product of the decarboxylation half-reaction (Fig. 6A). We cultured the strains in the presence of AIB and we demonstrated that both CML235-DGD1-Sk and CML235-DGD1-Su strains consume AIB, and after 48 h they produced stoichiometric amounts of acetone compared to the S. cerevisiae lab strain CML235-LacZ (Fig. 6B). Moreover, to demonstrate that the end product of the Dgd1p reaction is alanine, and then incorporated into the nitrogen metabolism, we disrupted the alanine aminotransferase gene ALT1 [34] in both S. kudriavzevii IFO1802 and S. uvarum AQ2901 strains, since it showed the best growth phenotype among all tested Saccharomyces isolates. Indeed, the mutant Sk-ALT1Δ showed a huge growth reduction in the presence of AIB. However, normal growth was observed in the mutant Sk-DGD1Δ growing in the presence of alanine (Fig. 6C). This confirms that the consumption of AIB as a nitrogen source follows the proposed pathway (Fig. 6C). All these results confirm that the gene DGD1 encodes a yeast dialkylglycine decarboxylase.

Fig. 5
figure 5

DGD1-carrying CML235 growth curves and Dgd1 protein production. A The cells were cultured in 200 µL of minimal medium (YNB, 10 mM AIB, 10 mM proline, 1% raffinose as carbon source, and 2% galactose as inducer) at 25 °C. On the right, a plot of the maximum specific growth rates (µmax) is shown. The error bars are standard deviations based on three biological replicas. Statistical differences were obtained through an ANOVA analysis. The raw data, Gompertz model fitting, and statistical analyses are given in Additional file 11. B Protein production profile at different time points after overnight cultures were transferred to the inducer medium. The V5-labelled Dgd1p and lacZ proteins were detected by horseradish peroxidase (HRP)-conjugated anti-V5 primary antibody. The loading protein control Tdh3p was detected by Anti-Tdh3p primary antibody coupled with an HRP-conjugated anti-mouse secondary antibody. Protein production is equal to the Dgd1p/LacZ peak band area divided by the Tdh3p peak band area. The Western blot raw data, the experimental molecular weight of the Dgd1p produced by the expression of the S. uvarum and S. kudriavzevii DGD1 alleles, and the molecular weight calibration are given in Additional file 11

Fig. 6
figure 6

Saccharomyces in vivo Dgd1 activity. A Decarboxylation half-reaction is carried out by dialkylglycine decarboxylase [13, 14]. B Growth and AIB consumption curves showed by the induced protein producer strains (left), AIB consumption, and acetone production after 48 h (right). C alt1 IFO1802 mutant is unable to grow in the presence of AIB. Ala: 10 mM L-alanine; Gln: 10 mM L-glutamine; AIB: 10 mM 2-aminoisobutyric acid. The error bars are the standard deviation of three biological replicas. Statistical differences were obtained through one-way ANOVA analysis. The raw data and statistical analyses are given in Additional file 12

DGD2 encodes a putative zinc-cluster regulatory protein

Since the strains Sk-TF and Su-TF (hereafter named Sk-DGD2 and Su-DGD2) lost their ability to grow in the presence of AIB and showed an impaired resistance against AIB (Fig. 4), we hence analyzed the sequence of the novel gene DGD2.

We first observed that the lengths of the different deduced amino acid sequences derived from the alleles were variable, between 551 and 625 residues (Fig. 7A). CR85 possesses the larger Dgd2p sequence and is the only one exhibiting a distinguishable fungal zinc finger Zn2Cys6 motif at the Nt end, according to the PROSITE database. Therefore, we performed a manual search upstream of the annotated start codons of the other available genome sequences of the S. kudriavzevii (CBS12357, CA111, CBS12751, and IFO1802) and S. uvarum strains (NPCC1290, BMV58, CBS7001, and NPCC1314) with shorter coding regions, and, despite these regions contained a putative Zn2Cys6 motif similar to that of CR85, the absence of start codons before the domain and the presence of stop codons in this region for all sequences indicated that these regions are pseudogenized in all strains except CR85 (Fig. 7A). To confirm this observation, we sequenced the DNA region corresponding to the zinc finger Zn2Cys6 of the S. kudriavzevii strains IFO1802 and AQ2901 and confirmed the presence of stop codons in that region (data not shown). Therefore, due to the pseudogenization of the 5′ end of the DGD2 gene of all strains, except CR85, their Dgd2p proteins are translated from other downstream methionine start codon, resulting in shorter Dgd2 proteins lacking the Zn2Cys6 motif at the amino end.

Fig. 7
figure 7

Dgd2p functional region determination. A Up, a general view of the positions of the identified functional sites in the CR85 Dgd2p compared to the other Dgd2p. Down, alignment of the available Saccharomyces Dgd2p amino acid sequences deduced from the orthologous nucleotide sequence, using CR85 as a reference. The upper green lines of each sequence indicate the encoded Dgd2p sequences according to the gene annotations. It can be observed that in most strains the methionines of the start codons are located 60–74 codons downstream of the start codon of CR85. When this homologous region of 60–74 codons is translated in the other strains, the start codon of CR85 is absent, and stop codons appear, indicating that this region is pseudogenized in all strains except CR85. B Alignment of the middle homology region (MHR) of S. cerevisiae zinc binuclear proteins with the CR85 Dgd2p sequence. (*) The conserved MHR amino acids were described elsewhere [35]. C Alignment of the S. cerevisiae Cha4p activation domain (AD) with the CR85 Dgd1p C-terminal region. D Identity of each Saccharomyces Dgd2p and the consensus amino acid sequence with respect to S. cerevisiae Cha4p. The numbers in the brackets indicate the amino acid positions of Chap4p referred to the start codon of CR85 Dgd2p

In addition, the alignment of the CR85 Dgd2p with other S. cerevisiae zinc binuclear cluster proteins (the closely related Cha4p, as well as Put3p, Prpr1p, Pdr1p, Leu3p, Gal4p, and Dal81p) allowed us to identify the core part of the middle homology region motif (MHR) [35] located at the position 297–378 of Dgd2p (Fig. 7B). Moreover, Dgd2p also contains a region at C-terminal similar to the Cha4p activation domain (AD) (Fig. 7C) [35, 36]. Besides, the consensus Dgd2p, starting from the zinc finger motif sequence, showed 42.3% identity with the S. cerevisiae Cha4p. Identity was even higher in the individual Dgd2p sequences (Fig. 7D). Although the Zn2Cys6 is absent in most strains, the MHR and AD domains are present in Dgd2p from all S. uvarum and S. kudriavzevii strains. Thus, the above data suggest that the gene DGD2 might encode a putative regulatory protein that specifically regulates the expression of DGD1 in the presence of AIB, but regulation may be different in CR85 for the rest of the strains.

The gene DGD2 is required to induce the expression of the DGD1 gene in the presence of 2-aminoisobutyric acid

To validate the function of Dgd2p as the regulator of DGD1, we cultured the wild-type strains S. kudriavzevii IFO1802 and S. uvarum AQ2901, and their dgd2 mutants Sk-DGD2Δ and Su-DGD2Δ in a minimal medium with AIB. We previously determined that 1 mM AIB was the optimal concentration to culture both Sk-DGD2Δ and Su-DGD2Δ strains to reduce the impact of its growth inhibitory effect (Additional file 6: Fig. S5). When cell concentrations reached 1 × 107 cells/mL, we extracted the total RNA to generate cDNA, to quantify the relative expression of DGD1 by qPCR, using genes the actin gene ACT1 and 18S rRNA as references. We observed a 65-fold and 104-fold induction of DGD1 in the S. kudriavzevii IFO1802 and S. uvarum AQ2901 strains when they were cultured in the AIB medium plus proline compared to the value expression obtained in proline (Fig. 8, AIB + P vs P). These results confirm a specific induction of DGD1 in the presence of AIB. However, we observe slight and no differences between the expression values obtained in AIB plus glutamine and glutamine in the strains AQ2901 and IFO1802, respectively (Fig. 8, AIB + G vs G). Interestingly, we observed a 26-fold and 128-fold induction in the AIB plus proline condition compared with the AIB plus glutamine condition in the strains IFO1802 and AQ2901, respectively (Fig. 8, AIB + G vs AIB + P). The latter result agrees with an inducer exclusion of DGD1. Finally, the ability to induce the expression of DGD1 in the presence of AIB is lost in both mutant strains Sk-DGD2Δ and Su-DGD2Δ, in comparison to their parental strains IFO1802 and AQ2901, which showed a 33-fold and 31-fold induction of DGD1, respectively (Fig. 8, AIB + P). These results confirm that the gene DGD2 encodes the positive regulator of DGD1 required to induce the AIB-dependent expression of DGD1.

Fig. 8
figure 8

DGD1 relative expression. The expression values of DGD1 in the strains IFO1802 and AQ2901 and their dgd2 mutants Sk-DGD2∆ and Su-DGD2∆ for each treatment are shown. The fold change represents the log-2 base of the relative expression of DGD1, normalized by the average expression of the reference genes ACT1 and 18S rRNA divided by the average of the relative expression of all treatments. G: 10 mM Glutamine; P: 10 mM Proline; AIB: 1 mM 2-aminoisobutyric acid. The error bars are the standard deviation of three biological replicas. Statistical differences were obtained through 2-way ANOVA analysis. The raw and relative expression data, and statistical analyses are given in Additional file 13

On the origin of the Saccharomyces genes DGD1 and DGD2

We identified the function of the genes DGD1 and DGD2, which are needed to catabolize AIB. Since the dialkylglycine decarboxylase enzyme has been identified in bacteria and filamentous fungi [8,9,10], we searched for orthologues of the three genes DGD1, DGD2, and APP of the subtelomeric cluster in the available 313 genome sequences of different species of the subphylum Saccharomycotina [4] to subsequently perform phylogenetic and synteny analyses (Fig. 9A and Additional file 7: Fig. S6). In the case of the yet-unidentified AAP gene, we could not find orthologues nor possible related genes adjacent to DGD1 or DGD2. In this way, we should remark that the presence of orthologous genes is conclusive, but their absence is not. Except in the case of highly accurate long-read sequencing of some of the Saccharomyces species, these genes can be unrepresented in the genome assemblages based on short-read sequencing due to their subtelomeric position or, in the case of genomes from yeasts belonging to lineages very distant to Saccharomyces, could be missed during the search due to low levels of similarity.

Fig. 9
figure 9

DGD1 is present in other Saccharomycotina yeasts. A DGD1 phylogenetic tree, inferred by using the maximum likelihood method conducted in MEGA 11, based on the LG model. The tree with the highest log likelihood (− 11,476.87) is shown. A discrete Gamma distribution was used to model evolutionary rate differences among sites (+ G, parameter = 0.5623). The tree is drawn to scale, with branch lengths measured in the number of amino acid substitutions per site. Numbers on the nodes correspond to bootstrap values based on 500 replicates. Circles of different colors at the right of the yeast names indicate the phylogenetic clades they belong to according to previous yeast phylogenetic analyses and taxonomic proposals [4, 37]. B Growth phenotype of Zygosaccharomyces and Torulaspora isolates in the presence of AIB as the sole nitrogen source

Except for the three Saccharomyces species under study, we found that DGD1 (Fig. 9A) was only found in different yeast species belonging to lineages that diverged before the whole-genome duplication (pre-WGD) [38]. Moreover, Saccharomyces DGD1 genes clustered together with members of the Zygosaccharomyces/Torulaspora (ZT) clade [39], instead of forming a differentiated clade (Fig. 9A), and maintaining the same DGD1-DGD2 gene tandem order as Z. kombuchaensis, one of the closest species in the phylogeny (Additional file 7: Fig. S6), with an average divergence of 0.26 ± 0.01 nucleotide substitutions per site, compared to 0.30 ± 0.01 within Zygosaccharomyces, and 0.29 ± 0.01 between Saccharomyces and Zygosaccharomyces. The absence of this gene in post-WGD species, except for the three Saccharomyces species, the unexpected phylogenetic relationships within the ZT clade, and the conserved gene cluster synteny are evidence of a putative horizontal gene transfer event in the past.

In the case of the gene DGD2, the search for homologous genes in the available Saccharomycotina genome sequences resulted in the identification of CHA4 and DGD2 sequences due to their similarities, Cha4p and Dgd2p from Saccharomyces species showed a 44.8 ± 2.0% of average identity.

The subsequent phylogenetic analysis, based on their encoded proteins, showed that CHA4 and DGD2 are paralogous genes that were duplicated before the divergence of the Saccharomycetaceae yeasts (Additional file 7: Fig. S6). It is interesting to remark that the ancestral gene block order with DGD1 has only been preserved in some Lachancea species, as DGD1-CHA4, and in Z. kombuchaensis, as DGD1-DGD2, even when the latter also contains a CHA4 gene.

CHA4 was preserved in most species of this family and the phylogenetic relationships shown by the CHA4 gene clade are compatible with the Saccharomycetaceae species tree [4, 37, 40]. Contrastingly, the DGD2 gene was only found in a few species of the ZT clade, T. microellipsoides, Z. rouxi, and Z. kombuchaensis. The Dgd2p of Z. kombuchaensis is the closest to the Saccharomyces Dgd2p (54.3% ± 1.9% of average identity), and this species is the only ZT clade taxon that maintains the same DGD1-DGD2 synteny. These results reinforce the horizontal gene transfer hypothesis to explain the origin of the Saccharomyces DGD1-DGD2 cluster.

Alternative explanations to the HGT (hypothesis 1): DGD2 appeared as a duplication of CHA4 in the ZT clade, and then transferred to Saccharomyces yeasts (hypothesis 2), or as a duplication of CHA4 in the Saccharomyces genus and then transferred to the ZT clade species (hypothesis 3), were tested with the Shimodaira-Hasegawa [41], the one-sided Kishino-Hasegawa [42], and the Expected Likelihood Weight [43] methods based on likelihood estimates. Hypothesis 1 (lnL -37,378.68, p-values 1.000, 1.000, 0.957, respectively) was the best, and hypotheses 2 (lnL -37,411.72, p-values 0.036, 0.026, 0.020, respectively) and 3 (lnL -37,448.18, p-values 0.000, 0.000, 0.000, respectively) were worse and rejected.

The massive, independent DGD2 gene losses required to explain the absence of DGD2 in Saccharomycestaceae species are compatible with different pseudogenization events, likely due to loss of function, as observed among the Saccharomyces species under study.

Because Saccharomyces DGD1 genes clustered with pre-WGD yeast of the ZT clade, we tested if our available Zygosaccharomyces and Torulaspora isolates (Table 1) were able to grow in the presence of AIB as the sole nitrogen source. Thus, the Zygosaccharomyces rouxii CECT1232 isolate showed slow growth in the presence of AIB. In contrast, the Torulaspora isolates grew well in the presence of AIB (Fig. 9B), being strain CBS6762 the one that exhibited the best growth phenotype.

All these results suggest that many pre-WGD yeast species exhibit dialkylglycine decarboxylase activity and the Saccharomyces DGD1 might have been acquired from an ancient horizontal gene transfer event from a member of the ZT clade.


In this study, we identified a novel subtelomeric Saccharomyces gene cluster found in the species S. uvarum, S. kudriavzevii, and S. eubayanus, composed of three genes, of which we could characterize two of them, named DGD1 and DGD2. We demonstrated that these two genes are involved in the catabolism of the non-proteinogenic amino acid 2-aminoisobutyric acid (AIB). DGD1 encodes a yeast dialkylglycine decarboxylase enzyme initially identified by the presence of an aminotransferase class III PLP-binding site [11], the high identity showed with the Burkholderia cepacia dialkylglycine decarboxylase gene (DGDA) [8], and the ability of the Saccharomyces isolates possessing the DGD1 gene to grow in the presence of AIB as a sole nitrogen source, although their phenotypes were variable both at the interspecific and intraspecific levels.

Deletants derived from strains S. kudriavzevii IFO1802 and S. uvarum BMV58, exhibiting the best AIB growth, were generated to validate DGD1 as the gene responsible for the alkylglycine decarboxylase activity. Because the BMV58 strain initially exhibited a slow growth, we also tested an alternative way to assay the dialkylglycine decarboxylase activity which is based on the ability of yeasts to resist the inhibitory growth effect exerted by AIB, as reported by Kim and Roon [17]. The impaired growth and null resistance against AIB exhibited by the mutants Sk-DGD1∆ and Su-DGD1∆, compared with their parental strains, indicate that AIB exerts toxicity inside the cell and support that the gene DGD1 encodes a dialkylglycine decarboxylase activity involved in the metabolization of the toxic AIB. Concordantly, the inhibitory effect of AIB was strong in the presence of proline, a “poor” nitrogen source, but insignificant in the presence of glutamine, a preferred nitrogen source. This experiment also demonstrates that the general amino acid permease Gap1p mediates the uptake of AIB into the cell. In the presence of a poor nitrogen source, such as proline, Gap1p is transporting AIB, but in the presence of glutamine, a preferred nitrogen source, GAP1 is repressed and the uptake of AIB is not possible [17, 44]. Differences in the toxicity susceptibility or the AIB uptake may also explain the differences observed in the growth of the different Saccharomyces strains when AIB was the sole nitrogen source.

Finally, AIB consumption and the acetone production from AIB, which is the by-product of the first decarboxylation half-reaction, also demonstrated that DGD1 encodes a yeast dialkylglycine decarboxylase enzyme. Both AIB usage and acetone production specifically underline dialkylglycine decarboxylase activity [9, 10, 45]. Moreover, the reduced growth of the mutants Sk-ALT1Δ and Su-ALT1Δ in the presence of AIB confirmed that the genes involved in the use of AIB as a nitrogen source are DGD1 and ALT1.

Surprisingly, we observed similar impaired phenotypes in the dgd2 mutants. Therefore, we analyzed the deduced amino acid sequence of the protein encoded by DGD2. We found a zinc finger Zn2Cys6 motif, which is only conserved in the S. kudriavzevii CR85 strain but is absent in the other strain sequences according to their shorter 5′ end of their coding regions. In the other strains, the homologous Zn2Cys6 motif region is pseudogenized (absence of the original star codon and the presence of stop codons) and Dgd2p is translated from an alternative star codon located 60 codons (74 in the case of IFO1802) downstream of the original one. In Saccharomyces, genes located in subtelomeric regions are recombinogenic and subjected to a higher mutation rate, and hence, can become totally or partially pseudogenized [46].

Although the DBD’s metal biding portion is essential for the DNA binding activity, it can be dispensable in some cases and still exerts its regulatory activity [15]. In particular, the expression of a truncated-zinc Zn2Cys6 finger motif DAL81 allele in a dal81 S. cerevisiae strain recovers its ability to induce the urea amidolyase activity, encoded by the Dal81p-regulated DUR1,2 gene [47]. The same was observed when the expression of a truncated DAL81 allele lacking the six cysteine residues of the Zn2Cys6 finger motif could recover the ability of a dal81 mutant to express the β-galactosidase reporter under the control of the GABA upstream activation sequence (UASGABA), which is present in the promoters of both Dal81p- and Uga3p-regulated genes UGA1 and UGA4 [48]. Similarly, the mutation of the fourth cysteine residue of the Zn2Cys6 finger motif in the Aspergillus nidulans tamA gene, which is homologous to the S. cerevisiae DAL81 gene, did not impact on protein’s function, confirming that this motif is not required for its regulatory function [49]. The same behavior was observed in the regulatory protein Gcr1p, where the expression of a truncated GCR1 allele lacking its DBD could recover the wild-type phenotype of a gcr1 mutant [50]. In addition, the alignment of the CR85 Dgd1p sequence with other reported zinc binuclear cluster proteins allowed us to identify the characteristic functional domains shared by the members of this family [15, 35]. The middle homology region (MHR) domain in Dgd1p, which is believed to regulate the transcriptional activity of these proteins [35] and the region similar to the reported Cha4p activation domain (AD) at the C-terminal position, needed to recruit the transcriptional machinery into the promoter of the regulated target gene [51].

Despite the absence of the Zn2Cys6 finger motif, we demonstrated an AIB-dependent induction of the DGD1 gene. The null induction observed in the wild-type strains grown in the presence of AIB plus glutamine instead of proline was probably because AIB is not being transported into the cell since glutamine represses the activity of the permease Gap1p [44], and hence, the AIB uptake. A similar phenotype was observed in the double mutant gap1 agp1, which is defective in the uptake of tryptophan into the cell, and showed an expression reduction of 75% of the Aro80p-regulated ARO9 gene in the presence of its inducer tryptophan [52]. Therefore, the results agree with an inducer exclusion of DGD1, meaning that AIB must be uptaken into the cell before initiating the expression of DGD1. Besides, the inability to express DGD1 in both dgd2 mutants Sk-DGD2Δ and Su-DGD2Δ in the presence of AIB confirmed that DGD2 is required for the AIB-dependent induction of DGD1.

The absence of the Zn2Cys6 motif in the tested strains (S. kudriavzevii IFO1802 and S. uvarum AQ2901), however, has arisen the question of how the encoded Dgd2p from these alleles regulate the expression of DGD1. Moreover, the poor growth and basal DGD1 expression exhibited by the dgd2 mutant suggest the involvement of other unidentified regulatory elements. We observed that the similarity between Dgd2p and the regulatory Cha4p was 43–45%. Cha4p requires the coactivator complexes SAGA and Swi/Snf to regulate its target genes CHA1 and SER3 in response to serine and threonine [36, 53]. The long segments conserved across Dgd2p compared to those of Cha4p suggest that this protein might interact with some of these complexes in the presence of AIB to induce the expression of DGD1. Besides, both Gcr1p and Dal81p, where their DBD is dispensable, bind as heterodimers with the target proteins Rap1 and Dal82, respectively. The two latter proteins confer the required DBD for binding into the promoters of their target genes [50, 54]. In addition, some members of the zinc binuclear protein family act as nutrient sensors, interacting either in or directly with the target nutrient such as the well-reported Gal4p and Put3p, respectively [16]. Therefore, a similar mechanism might be working on Dgd2p, which senses the intracellular AIB, producing a conformational change that allows the recruitment of the transcriptional machinery, but binds into the DGD1 promoter as a heterodimer with a yet-unidentified protein that confers the DNA binding activity.

Although we characterized the function of the genes DGD1 and DGD2, their origins and physiological roles in nature were unclear. We found orthologues of both genes in the other Saccharomycotina yeasts, where the synteny was conserved in several pre- and post-WGD clade species. In addition, we demonstrated that some isolates from the ZT and KLE clades exhibited dialkylglycine decarboxylase activity. Both Saccharomyces DGD1 and DGD2 clustered within the ZT clade, instead of forming their differentiated clade in contrast to the species phylogeny [4, 37, 40]. The unexpected phylogenetic position, the identical gene order, and the absence of these genes in other post-WGD species are clear evidence of a horizontal gene transfer event [1, 2, 5] from a member close to Zygosaccharomyces. Gene acquisition from non-Saccharomyces donors has also been reported in wine S. cerevisiae strains [3, 6], including the gene FSY1 [7], which was also lost in the post-WGD species [55] and, later, horizontally transferred to S. cerevisiae [6].

A reported great source of AIB is the fungal antimicrobial oligopeptides known as peptaibols, which contain high levels of AIB (~ 56%), giving them a hydrophobic helix conformation, and therefore, increased stability and resistance against proteases [12, 56]. A variety of peptaibols has been identified in Trichoderma species, and many studies have proposed their use as biocontrol agents against pathogenic fungal microorganisms [57, 58].

Moreover, isovaline, another dialkylamino acid found in the structure of the peptaibols [12], was reported as an inducer of the DGDA activity [8], and can also be consumed by those yeasts with dialkylglycine decarboxylase activity (Additional file 8: Fig. S7). Since peptaibol-producing fungi are found in many natural niches [58] and Zygosaccharaomyces isolates are widespread in the same natural environments (soil, decayed leaves, and tree bark) as the wild Saccharomyces non-cerevisiae species [31], together with the findings obtained in this study, this prompted us to propose that these wild Saccharomyces yeasts acquired both DGD1 and DGD2 from an ancient member close to the Zygosaccharomyces genus, as part of detoxification mechanism through the catabolism of AIB, a by-product of the peptaibol degradation. Later, these genes could be lost in the evolutionary more recent Saccharomyces species, perhaps due to loss of function during the colonization of new habitats, such as sugar-rich substrates and fermentation environments where peptaibols are absent.


In this study, we identified and characterized the novel Saccharomyces genes DGD1 and DGD2 which encode a yeast dialkylglycine decarboxylase enzyme and its AIB-responsive positive regulator, respectively, that are involved in the catabolism of AIB. The Dgd2p exerts its regulatory function despite the absence of its DBD motif which suggests the involvement of other regulatory proteins. The phylogenetic analysis indicated that both genes might have been acquired through HGT from a yeast closely related to the Zygosaccharomyces clade. Our results suggest that these genes could confer a detoxification mechanism against the inhibitory effect of AIB, which can be released as a potential degradation product of peptaibols produced by fungi in natural environments. Future experiments will address cis-regulatory elements of DGD1, the Dgd2p functional domain, and how the proposed regulatory proteins interact with Dgd2p to promote de AIB-dependent induction of DGD1.


Yeast strains

All the wild strains used in this study are listed in Table 1. These strains were grown on YPD solid medium plates (1% yeast extract, 2% peptone, 2% glucose, 2% agar) and maintained at 4 °C for further experiments.

Identification of novel genes in Saccharomyces species

Both S. uvarum CBS7001 and S. kudriavzevii IFO1802 genomes [59] were re-annotated following a combination of two approaches as described elsewhere [60], which revealed a novel cluster of three unknown genes. A blastx search [61] of the three genes against the non-redundant protein sequence database was performed in other S. uvarum and S. kudriavzevii strains and S. eubayanus CBS12357 [62]. Simultaneously, a blastn search against both the non-redundant database and Saccharomyces assemblies (Additional file 1: Table S1) was carried out to check either the presence or absence of these genes. The discovered aminotransferase-like protein (AT) and putative zinc finger transcription factor (TF) gene sequences in the S. kudriavzevii strains IFO1802, CA111, CBS12751, and CR85; S. uvarum strains NPCC1290, NPCC1314, CBS7001, BMV58, and S. eubayanus strain CBS12357 were translated to their deduced amino acid sequence with the Geneious Prime® 2020.2.4 software using the standard code. The sequences were aligned with the Clustal Omega 1.2.2 tool using the default parameters, and a consensus sequence was extracted. A search for documented protein domains was performed through the InterProScan [63] tool of Geneious Prime® 2020.2.4 software against the PROSITE database and a blastp search against the Swissprot database was carried out with default parameters using a max E-value equal to 0.1. Then, we extracted the sequence with the highest identity, and we carried out a new alignment with the Clustal Omega 1.2.2 tool.

Zinc finger DNA region sequencing

A 600-bp PCR product that covers the DGD2 zinc finger motif DNA sequence (approximately 300 bp upstream from the annotated sequence) was amplified from total DNA extracted from AQ2901 and IFO1802 strains using Phusion™ High-Fidelity Polymerase (Thermo Scientific) following the provider instructions employing sequencing primers (Table S6). They were loaded into 2% agarose gel, rescued, and purified through MinElute® PCR purification Kit (Qiagen). The fragments were sequenced through the University of Valencia Experimental Research Support Central Service’s Sanger sequencing (SCSIEUV, Spain) using the sequencing primers.

Growth phenotype screening

The Saccharomyces strains (Table 1) were used to assay their ability to grow in the presence of 2-aminoisobutyric acid (AIB) as the sole nitrogen source. Precultures were incubated overnight in liquid YNB medium (0.17% yeast nitrogen base without amino acid and ammonium, 2% glucose, 5 g/L (NH4)2SO4) at 25 °C. Then, cells were grown on YNB plates (0.17% yeast nitrogen base without amino acid and ammonium, 2% glucose, 2% agar) containing three different AIB (Sigma Aldrich, Saint Louis, MO) concentrations (1, 5, and 10 mM) at 25 °C. Growth on YNB solid media containing 10 mM glutamine (Sigma Aldrich, Saint Louis, MO) was used as a control.

Usage of isovaline as a nitrogen source

IFO1802 wild-type strain and their dgd1 and dgd2 mutants were plated on YNB solid media containing 10 mM L-isovaline (Thermo Fisher Scientific, Waltham, MA, USA) either as the sole nitrogen or plus 10 mM proline (Aditional file 8: Fig. S7). The plates containing 10 mM proline, AIB, and AIB plus proline were used as control media.

Mutant strain construction

The mutant strains generated, and the primers used in this study are listed in Tables 2 and 3, respectively. The S. uvarum strain AQ2901 is a haploid derivate of the commercial wine strain BMV58 (Lallemand, Montreal, Canada). Strains AQ2901 and IFO1802 were transformed using the lithium acetate method changing the thermal shock to 37 and 34 °C, respectively [64]. The deletions of the subtelomeric individual genes and the entire cluster in the AQ2901 strain were carried through PCR-mediated gene disruption using the NATMX4 cassette as a selection marker [65]. The NATMX4 cassette was PCR amplified from the pAG25 plasmid [66] using NZYTaq II DNA Polymerase (NZYTech, Lisbon, Portugal) following the supplier’s instructions and employing deletion primers (Table 3), whereas the cassette KANMX from the plasmid pUG6 [67] was used for the deletion of the ALT1 gene and was amplified with the corresponding deletion primers (Table 3) under the same conditions mentioned above. Total DNA was extracted from antibiotic-resistant transformants which grew on a selective YPD solid medium (1% yeast extract, 2% peptone, 2% glucose, 2% agar, 100 µg/mL nourseothricin or 200 µg/mL G418) at 25 °C after 4 days and gene deletions were confirmed by PCR analysis using the diagnostic primers (Table 3).

Table 3 Primers used in this study

Deletion of the four copies of the subtelomeric genes and the two ALT1 alleles in the S. kudriavzevii diploid strain IFO1802 was performed through CRISPR-Cas9 gene disruption [68]. The protospacer sequences were chosen according to [69], implementing the IFO1802 genome sequence as a reference to avoid selecting unspecific gRNA. Then, we amplified by PCR the whole pRCC-N plasmid by PCR which carries the natMX resistance marker with primers carrying the protospacer sequence at their 5′ ends [70]. The PCR was carried out with Phusion™ High-Fidelity Polymerase (Thermo Scientific, Vilnius, Lithuania) using the protospacer-carrying primers (Table 3). Before the addition to the transformation mix, 30 µL of the PCR product was treated with 10U of DpnI (Thermo Scientific, Vilnius, Lithuania) for 3 h to guarantee the total degradation of the pRCC-N original template. To ensure DNA reparation by homologous recombination, we used a double-stranded 80-bp oligonucleotide as donor DNA (dDNA), with 40 nucleotides on either side that are homologous to both upstream and downstream sequences of the target gene, respectively [71]. The oligonucleotides were assembled by mixing equal molar amounts of two complementary single-stranded 80-bp oligonucleotides (Table 3), heating the mix to 99 °C for 5 min, and subsequently, cooling down to 25 °C at a rate of 0.1 °C/s. One nanomole of the double-stranded oligonucleotide was added to the transformation mix, and the gene deletions were confirmed by PCR analysis using total DNA extracted from nourseothricin-resistant transformants, using the corresponding diagnostic primers (Table 3).

Mutant strain phenotyping

The generated mutant strains of AQ2901 and IFO1802 (Table 2) were incubated overnight in a liquid YNB medium at 25 °C, and then, cultivated on YNB plates containing 10 mM AIB as the sole nitrogen source. The resistance against the AIB growth inhibitory effect was also assayed [17]. Briefly, cells were plated on YNB solid media containing 10 mM AIB plus either 10 mM proline (Sigma Aldrich Saint Louis, MO) or 10 mM glutamine. Growth on YNB plates containing only either 10 mM proline or 10 mM glutamine as the sole nitrogen source were used as controls. Similarly, the alt1 mutant was incubated on YNB plates containing either 10 mM AIB, 10 mM L-glutamine, or 10 mM L-alanine (Sigma Aldrich Saint Louis, MO).

DGD1 cloning

DGD1 genes were amplified from the genomic DNA of IFO1802 and AQ2901 strains using the cloning primers (Additional file 9: Table S2). The PCR was carried out using TaKaRa Ex Taq™ polymerase (Takara, Kusatsu, Shiga, Japan) following the supplier’s instructions. The DGD1-IFO1802 PCR product was purified through the MinElute® PCR purification Kit (Qiagen, Hilden, Germany). Before the cloning step, 1 µg of DGD1-IFO1802 PCR product was treated with 10 U XcmI (New England BioLabs®, Ipswich, MA, USA) in NE Buffer 2.1 to digest the indel-containing DGD1 copy amplified from chromosome X. The digestion product was loaded into an agarose gel, and the non-digested band corresponding to the chromosome VII copy was rescued and purified with the MinElute® PCR purification Kit (Additional file 2: Fig. S1). The DGD1-AQ2901 was purified with the High Pure PCR Purification Kit (Roche, Mannheim, Germany) to discard the small unspecific band (Additional file 3: Fig. S2). Both DGD1 genes were inserted into the pYES2.1 TOPO® TA plasmid (Invitrogen, Waltham, MA, USA) and cloned into E. coli TOP10F’ strain (Invitrogen Waltham, MA, USA). The transformant E. coli strains (Additional file 9: Table S3) were selected on Ampicillin LB plates (1% tryptone, 0.5% yeast extract, 1% NaCl, 2% agar, 100 µg/mL ampicillin). The right orientation of the DGD1 inserts was checked through the analysis of the restriction fragment length pattern obtained from the digestion of the DGD1-carrying plasmids (Table 4). The plasmids carrying the AQ2901 DGD1 allele were digested with PvuII (Fermentas Waltham, MA, USA) in buffer G, and those carrying the Chromosome VII IFO1802 allele were double digested with PvuII and SphI (Invitrogen, Waltham, MA, USA) in buffer G. Once the right DGD1 orientation was confirmed in both plasmids (Additional files 4 and 5: Figs S3 and S4, respectively), the sequences of the inserts were obtained by Sanger sequencing using sequencing primers (Additional file 9: Table S2), at the Genomics Section of the Central Service of Experimental Research Support (SCSIE), University of Valencia, Spain. The haploid S. cerevisiae CML235 strain, which is a spore-derivative from the strain FY1679, was used as the host cell for recombinant protein production. The strain was transformed with 400 ng of the constructed plasmids pYES-Sk-DGD1 and pYES-Su-DGD1 (Table 4) using the lithium acetate method and the transformants were selected on a solid SC drop-ura medium (0.67% yeast nitrogen base without amino acid, 1.93% p/v synthetic complete drop-out [Formedium], 2% glucose, 2% agar) and the plasmid pYES-LacZ (Table 4) was used as the plasmid control.

Table 4 Plasmids used in this study

Growth phenotype of CML235 strains carrying the DGD1 genes

To test the growth phenotype in the presence of AIB of the DGD1-carrying CML235 strains (Table 2), overnight precultures of the strains CML235-DGD1-Sk, CML235-DGD1-Su, and CML235-LacZ were carried out in SC drop-ura medium containing 2% raffinose, as carbon source instead of glucose. Then, they were inoculated in 200 µL of YNB liquid medium containing 10 mM AIB, 10 mM proline, required amino acid supplements for auxotrophies (500 mg/L histidine, 125 mg/L leucine) [72], 1% raffinose as carbon source, and 2% galactose for inducing the expression of DGD1, with an initial OD600 of 0.2 on 96 well-microtiter plates at 25 °C. Growth curves were monitored through OD measurements at 600 nm wavelength in a SPECTROstar Nano® microplate reader (BMG LABTECH). Growth curves were fitted to the Gompertz model by using the grofit R package [73], and maximum specific growth rates (µmax) were obtained.

Recombinant protein production kinetics

The strains CML235-DGD1-Sk and CML235-DGD1-Su were incubated in 15 mL of SC drop-ura containing 2% raffinose overnight at 30 °C, then the cells with an initial OD600 of 0.4 were inoculated in 100 mL of inducer medium (0.67% yeast nitrogen base without amino acid, 1.93% p/v synthetic complete drop-out, 1% raffinose, and 2% galactose) in 250-mL flasks at 30 °C with a shacking speed of 160 rpm. The strain CML235-LacZ was used as a recombinant protein control producer. The growth curves were followed at different times (0, 3, 6, 9, 12, and 24 h) through OD measurements at 600 nm wavelength using a Fisherbrand™ Cell Density Meter. Five-milliliter samples were taken, and the cell pellets were collected and frozen with liquid nitrogen and stored at − 80 °C until recombinant protein production analysis. Cell extracts were prepared according to a slightly modified post-alkaline extraction [74]. Briefly, cell pellets were resuspended in 200 µL of 0.2 M NaOH and incubated for 5 min at room temperature. Then they were pelleted and resuspended in 100 µL SDS-PAGE loading buffer (0.06 M Tris–HCL pH 6.8, 25% glycerol, 2% SDS, 14.4 mM β-mercaptoethanol, 0.1% bromophenol blue) and boiled for 5 min and pelleted again. Equal amounts of proteins were loaded and resolved in 12% SDS-PAGE gels and transferred to nitrocellulose membranes. Ponceau staining was used to confirm the correct protein transfer. The recombinant V5-tagged Dgd1 proteins were detected employing a horseradish peroxidase (HRP)-conjugated anti-V5 primary antibody (R96125; Invitrogen, Waltham, MA, USA). Anti-Tdh3p primary antibody (provided by Daniel Gonzalbo, University of Valencia) and HRP-conjugated anti-mouse secondary antibody (GE Healthcare Life Sciences, Chicago, IL, USA) were used to determine Tdh3p protein levels as the loading control. Pierce™ ECL Western Blotting Substrate (32,109, Thermo Scientific Waltham, MA, USA) was used for the detection of HRP-labelled proteins. Immunoblot images were obtained in an Amersham ImageQuant 800 system (Cytiva, Marlborough, MA, USA). Specific signals and peak band area quantifications were determined with ImageQuant TL software. Relative quantification of recombinant Dgd1p proteins at each time was calculated as the Dgd1p peak band area divided by the Tdh3p peak band area.

In vivo Dgd1p activity assay

Strains CML235-DGD1-Sk, CML235-DGD1-Su, and CML235-LacZ were incubated overnight in 20 mL of SC drop-ura containing 2% raffinose at 30 °C. Afterward, cell pellets were centrifugated at 3500 × g and the supernatant was discarded. Then, pellets were resuspended in 20 mL of inducer medium for 3 h. At that moment, the cell pellets were recovered again and washed once in 20 mL of YNB-AIB medium (10 mM AIB, 500 mg/L histidine, 125 mg/L leucine, 1% raffinose, and 2% galactose) and inoculated in 100 mL of YNB-AIB medium with an initial OD600 of 0.2 at 30 °C with 120 rpm of shacking. Growth curves were followed at different times through OD measurement at 600 nm wavelength using a Fisherbrand™ Cell Density Meter (Fisher Scientific, Madrid, Spain).

The residual AIB measurement was performed in an ultimate 3000®UPLC (Thermo Fisher Scientific, Waltham, MA, USA) equipped with a UV–visible detector (Thermo Fisher Scientific, Waltham, MA, USA). The method was based on [75] but adapted to our conditions. Four hundred-microliter samples were derivatized with a mix of 12 µL diethyl ethoxymethylenemalonate (DEEMM) and 300 µL methanol. The reactions were carried out in screw-cap test tubes in an ultrasonic bath for 30 min, followed by heating at 80 °C for 2 h to degrade the excess DEEMM, and filtrated using 0.22-µm nylon syringe filters (Labbox Labware, Barcelona, Spain). The chromatographic analyses were conducted with an Accuore™ C18 column (Thermo Fisher Scientific, Waltham, MA). The applied triphasic gradient, which consists of phase A (methanol), phase B (acetonitrile), and phase C (25 mM acetate buffer, pH 6.7), is shown in Additional file 9: Table S4. To quantify the acetone production, 5 mL of the sample was mixed with 5 mL of 300 g/L NaCl. Then passed through a TRACE™ GC Ultra gas chromatograph (Thermo Fisher Scientific, Waltham, MA, USA) coupled with a flame ionization detector (FID), equipped with a 30 m × 0.25 mm × 0.25 µm HP-INNOWax capillary column coated with a layer of cross-linked polyethylene glycol (Agilent Technologies, Santa Clara, USA) at carrier gas helium flow rate of 1 mL/min. The oven temperature program was as follows: (1) 5 min at 50 °C, (2) temperature raised to 100 °C at the increasing rate of 1.5 °C/min. (3) then up to 215 °C at a rate of 3 °C/min and (4) was kept for 2 min more. The FID detector temperature was at 280 °C and the acetone was identified by its retention time. Quantification was made through an acetone calibration plot.

DGD1 gene expression analysis by real-time qPCR

To determine whether DGD1 expression is regulated by the gene DGD2 and the amino acid AIB, strains BMV58 and IFO1802 and their dgd2 mutants were cultured overnight in 5 mL of YNB liquid medium. The cells were shed once with a YNB medium without any nitrogen source. Then, they were inoculated into 50 mL YNB liquid medium in 250 mL flasks containing 1 mM AIB plus either 10 mM glutamine or 10 mM proline with an initial cell concentration of 1 × 106 cells mL−1. YNB liquid medium containing either 10 mM glutamine or 10 mM proline as the sole nitrogen source was used as control media. Samples were taken when the cell concentration reached up to 1 × 107 cells mL−1, frozen with liquid nitrogen, and stored at − 80 °C until mRNA extraction. Total RNA from the frozen samples was extracted using the QIAGEN RNA extraction kit. The total RNA samples were treated with 10 U of DNase I (Roche) and the cDNA was generated from 200 ng of total RNA using the NZY First-Strand cDNA synthesis kit (NZYTech, Lisbon, Portugal). The qPCRs were performed in a LightCycler® 480 Instrument (Roche, Mannheim, Germany) using the qPCR primers (Table 3). The expression of DGD1 was normalized against the average expression of the reference genes ACT1 and 18S rRNA. Then, each sample value was relativized against the average value of all samples and transformed into a log-2 value.

To determine the optimal AIB concentration for the expression experiment, the mutant strains Su-DGD2Δ and Sk-DGD2Δ were plated on YNB medium at the three different AIB concentrations assayed previously (1, 5, and 10 mM) plus either 10 mM glutamine or 10 mM proline at 25 °C for 3 days. The mutant strains Su-DGD1Δ and Sk-DGD1Δ and their parental strains AQ2901 and IFO1802 were used as control.

Screening for orthologs in other yeast genomes

The sequences of three genes included in the cluster found in Saccharomyces (DGD1, DGD2, and AAP) were used to find orthologs in other yeast species. In total, 313 genome sequences of different species of budding yeasts [4] were used to run the genomic screening (Additional file 10: Table S5). A blastn [61] search was performed against the genomes with default parameters and word size set to 20. An in-house Python script was used to filter results by keeping hits with a total alignment length greater than 200 bp. Open-reading frames (ORFs) from the hits found were extracted and the longest ORFs for each gene were selected for further analysis. The translated sequences of the final selected ORFs were used to validate results by aligning against the Uniprot reference database ( using Blastp tool. We also studied whether synteny was conserved when two of three genes of the cluster were found in the same yeast genome.

Phylogeny reconstruction and comparison

Final validated DGD1 and DGD2 ORFs were used for phylogeny reconstruction. Sequences were translated into amino acids and aligned with MUSCLE [76] implemented in the MEGA v. 11.0.13 program [77].

The best evolutionary protein models based on empirical frequencies of amino acid replacements were selected with ProtTest 3.4.2 [78], and the best-fitting model for the Ddg1p alignment was the LG model [79] with gamma-distributed rates with an α shape parameter of 0.5623, and for the Dgd2p/Cha4p alignment, the JTT model [80] with a gamma distribution of rates with an α shape parameter of 0.8115, a proportion of invariable sites of 0.032 and the observed amino acid frequencies. Maximum likelihood phylogenies were obtained, with the appropriate model, by using the MEGA v. 11.0.13 program [77], with 500 bootstrap replicates.

Alternative phylogenetic hypotheses were compared with the Shimodaira-Hasegawa [41], the one-sided Kishino-Hasegawa [42], and the expected likelihood weights [43] tests implemented in Tree-Puzzle 5.3.rc [81].

Availability of data and materials

Genome data used in this study are available in NCBI (Additional file 10: Table S5, see references therein). All data generated or analyzed during this study are included in this published article and its supplementary information files. For those results, based on three replicates, additional files containing the individual data values and their statistical analyses are provided, as indicated in the corresponding figure legends. All materials are also available upon request to the corresponding author.



Putative amino acid permease

ACT1 :

Actin gene


2-Aminoisobutyric acid

ALT1 :

Alanine aminotransferase gene


Aminotransferase-like protein

DGD1 :

Dialkylglycine decarboxylase gene

DGD2 :

AIB-responsive positive regulator gene

GAP1 :

General amino acid permease gene


Horizontal gene transfer


Transcription factor


Pyridoxal phosphate


  1. Richards TA. Genome evolution: horizontal movements in the Fungi. Curr Biol. 2011;21(4):R166–8.

    Article  CAS  PubMed  Google Scholar 

  2. Fitzpatrick DA. Horizontal gene transfer in fungi. FEMS Microbiol Lett. 2012;329(1):1–8.

    Article  CAS  PubMed  Google Scholar 

  3. Novo M, Bigey F, Beyne E, Galeote V, Gavory F, Mallet S, et al. Eukaryote-to-eukaryote gene transfer events revealed by the genome sequence of the wine yeast Saccharomyces cerevisiae EC1118. Proc Natl Acad Sci USA. 2009;106(38):16333–8.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  4. Shen XX, Opulente DA, Kominek J, Zhou X, Steenwyk JL, Buh KV, et al. Tempo and mode of genome evolution in the budding yeast subphylum. Cell. 2018;175(6):1533–45.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  5. Hall C, Brachat S, Dietrich FS. Contribution of horizontal gene transfer to the evolution of Saccharomyces cerevisiae Eukaryot Cell. 2005;4(6):1102–15.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  6. Marsit S, Mena A, Bigey F, Sauvage F-X, Couloux A, Guy J, et al. Evolutionary advantage conferred by an eukaryote-to-eukaryote gene transfer event in wine yeasts. Mol Biol Evol. 2015;32(7):1695–707.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  7. Galeote V, Novo M, Salema-Oom M, Brion C, Valério E, Gonçalves P, et al. FSY1, a horizontally transferred gene in the Saccharomyces cerevisiae EC1118 wine yeast strain, encodes a high-affinity fructose/H+ symporter. Microbiology. 2010;156(12):3754–61.

    Article  CAS  PubMed  Google Scholar 

  8. Keller JW, Baurick KB, Rutt GC, O’Malley MV, Sonafrank NL, Reynolds RA, et al. Pseudomonas cepacia 2,2-dialkylglycine decarboxylase. Sequence and expression in Escherichia coli of structural and repressor genes. J Biol Chem. 1990;265(10):5531–9.

    Article  CAS  PubMed  Google Scholar 

  9. Adachi K, Nelson GH, Peoples KA, DeZwaan TM, Skalchunes AR, Heiniger RW, et al. Sequence analysis and functional characterization of the dialkylglycine decarboxylase gene DGD1 from Mycosphaerella graminicola Curr Genet. 2003;43(5):358–63.

    Article  CAS  PubMed  Google Scholar 

  10. Esaki N, Watanabe M, Kurihara T, Soda K. Fungal thermostable α-dialkylamino acid aminotransferase: occurrence, purification and characterization. Arch Microbiol. 1994;161(2):110–5.

    Article  CAS  Google Scholar 

  11. Schiroli D, Peracchi A. A subfamily of PLP-dependent enzymes specialized in handling terminal amines. Biochim Biophys Acta. 2015;1854(9):1200–11.

    Article  CAS  PubMed  Google Scholar 

  12. Ramachander Turaga VN. Peptaibols: antimicrobial peptides from fungi. In: Joginder Singh V, Meshram MG, editors. Bioactive natural products in drug discovery. Singapore: Springer; 2020. p. 713–30.

    Google Scholar 

  13. Sun S, Zabinski RF, Toney MD. Reactions of alternate substrates demonstrate stereoelectronic control of reactivity in dialkylglycine decarboxylase. Biochemistry. 1998;37(11):3865–75.

    Article  CAS  PubMed  Google Scholar 

  14. Fogle EJ, Toney MD. Mutational analysis of substrate interactions with the active site of dialkylglycine decarboxylase. Biochemistry. 2010;49(30):6485–93.

    Article  CAS  PubMed  Google Scholar 

  15. MacPherson S, Larochelle M, Turcotte B. A fungal family of transcriptional regulators: the zinc cluster proteins. Microbiol Mol Biol Rev. 2006;70(3):583–604.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  16. Sellick CA, Reece RJ. Eukaryotic transcription factors as direct nutrient sensors. Trends Biochem Sci. 2005;30(7):405–12.

    Article  CAS  PubMed  Google Scholar 

  17. Kim KW, Roon RJ. Transport and metabolic effects of α-aminoisobutyric acid in Saccharomyces cerevisiae Biochim Biophys Acta - Gen Subj. 1982;719(2):356–62.

    Article  CAS  Google Scholar 

  18. Querol A, Huerta T, Barrio E, Ramon D. Dry yeast strain for use in fermentation of Alicante wines: selection and DNA patterns. J Food Sci. 1992;57(1):183–5.

    Article  CAS  Google Scholar 

  19. Sniegowski PD, Dombrowski PG, Fingerman E. Saccharomyces cerevisiae and Saccharomyces paradoxus coexist in a natural woodland site in North America and display different levels of reproductive isolation from European conspecifics. FEMS Yeast Res. 2002;1(4):299–306.

    CAS  PubMed  Google Scholar 

  20. Mortimer RK, Johnston JR. Genealogy of principal strains of the yeast genetic stock center. Genetics. 1986;113(1):35–43.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  21. Pérez-Torrado R, Oliveira BM, Zemančíková J, Sychrová H, Querol A. Alternative glycerol balance strategies among Saccharomyces species in response to winemaking stress. Front Microbiol. 2016;7.

  22. Naumov GI, Naumova ES, Lantto RA, Louis EJ, Korhola M. Genetic homology between Saccharomyces cerevisiae and its sibling species S. paradoxus and S. bayanus: electrophoretic karyotypes. Yeast. 1992;8(8):599–612.

    Article  CAS  PubMed  Google Scholar 

  23. Rodríguez ME, Pérez-Través L, Sangorrín MP, Barrio E, Lopes CA. Saccharomyces eubayanus and Saccharomyces uvarum associated with the fermentation of Araucaria araucana seeds in Patagonia. FEMS Yeast Res. 2014;14(6):948–65.

    Article  PubMed  Google Scholar 

  24. Rodríguez ME, Pérez-Través L, Sangorrín MP, Barrio E, Querol A, Lopes CA. Saccharomyces uvarum is responsible for the traditional fermentation of apple chicha in Patagonia. FEMS Yeast Res. 2017;17(1):fow109.

    Article  CAS  Google Scholar 

  25. Lopes CA, Barrio E, Querol A. Natural hybrids of S. cerevisiae × S. kudriavzevii share alleles with European wild populations of Saccharomyces kudriavzevii. FEMS Yeast Res. 2010;10(4):412–21.

    Article  CAS  PubMed  Google Scholar 

  26. Naumov GI, Naumova ES, Louis EJ. Two new genetically isolated populations of the Saccharomyces sensu stricto complex from Japan. J Gen Appl Microbiol. 1995;41(6):499–505.

    Article  CAS  Google Scholar 

  27. Naumov GI, Lee CF, Naumova ES. Molecular genetic diversity of the Saccharomyces yeasts in Taiwan: Saccharomyces arboricola, Saccharomyces cerevisiae and Saccharomyces kudriavzevii Antonie van Leeuwenhoek. 2013;103(1):217–28.

    Article  CAS  PubMed  Google Scholar 

  28. Nespolo RF, Villarroel CA, Oporto CI, Tapia SM, Vega-Macaya F, Urbina K, et al. An Out-of-Patagonia migration explains the worldwide diversity and distribution of Saccharomyces eubayanus lineages. PLOS Genet. 2020;16(5):e1008777.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  29. Kurtzman CP. Torulaspora. In: Kurtzman CP, Fell JW, Boekhout T, editors. The yeasts. 5th ed. The Netherlands: Elsevier; 2011. p. 867–74.

    Chapter  Google Scholar 

  30. Kurtzman CP, Robnett CJ, Basehoar-Powers E. Zygosaccharomyces kombuchaensis, a new ascosporogenous yeast from “Kombucha tea.” FEMS Yeast Res. 2001;1(2):133–8.

    Article  CAS  PubMed  Google Scholar 

  31. James SA, Stratford M. Zygosaccharomyces. In: Kurtzman CP, Fell JW, Boekhout T, editors. The Yeasts. 5th ed. The Netherlands: Elsevier; 2011. p. 937–47.

    Chapter  Google Scholar 

  32. Johnson B, Brown CM. A possible relationship between the fatty acid composition of yeasts and the ‘petite’ mutation. Antonie van Leeuwenhoek. 1972;38(1):137–44.

    Article  CAS  PubMed  Google Scholar 

  33. Winston F, Dollard C, Ricupero-Hovasse SL. Construction of a set of convenient Saccharomyces cerevisiae strains that are isogenic to S288C. Yeast. 1995;11(1):53–5.

    Article  CAS  PubMed  Google Scholar 

  34. García-Campusano F, Anaya VH, Robledo-Arratia L, Quezada H, Hernández H, Riego L, et al. ALT1-encoded alanine aminotransferase plays a central role in the metabolism of alanine in Saccharomyces cerevisiae Can J Microbiol. 2009;55(4):368–74.

    Article  PubMed  Google Scholar 

  35. Schjerling P, Holmberg S. Comparative amino acid sequence analysis of the C6 zinc cluster family of transcriptional regulators. Nucleic Acids Res. 1996;24(23):4599–607.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  36. Holmberg S, Schjerling P. Cha4p of Saccharomyces cerevisiae activates transcription via serine/threonine response elements. Genetics. 1996;144(2):467–78.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  37. Dujon BA, Louis EJ. Genome diversity and evolution in the budding yeasts (Saccharomycotina). Genetics. 2017;206(2):717–50.

    Article  PubMed  PubMed Central  Google Scholar 

  38. Wolfe KH. Origin of the yeast whole-genome duplication. PLoS Biol. 2015;13(8):1–7.

    Article  Google Scholar 

  39. Marcet-Houben M, Gabaldón T. Beyond the whole-genome duplication: phylogenetic evidence for an ancient interspecies hybridization in the baker’s yeast lineage. PLoS Biol. 2015;13(8):1–26.

    Article  Google Scholar 

  40. Kurtzman CP. Phylogenetic circumscription of Saccharomyces, Kluyveromyces and other members of the Saccharomycetaceae, and the proposal of the new genera Lachancea, Nakaseomyces, Naumovia, Vanderwaltozyma and Zygotorulaspora. FEMS Yeast Res. 2003;4(3):233–45.

    Article  CAS  PubMed  Google Scholar 

  41. Shimodaira H, Hasegawa M. Multiple comparisons of loglikelihoods with applications to phylogenetic inference. Mol Biol Evol. 1999;16:1114–6.

    Article  CAS  Google Scholar 

  42. Kishino H, Hasegawa M. Evaluation of the maximum likelihood estimate of the evolutionary tree topologies from DNA sequence data, and the branching order in Hominoidea. J Mol Evol. 1989;29:170–9.

    Article  CAS  PubMed  Google Scholar 

  43. Strimmer K, Rambaut A. Inferring confidence sets of possibly misspecified gene trees. Proc R Soc Lond B. 2002;269:137–42.

    Article  Google Scholar 

  44. Magasanik B, Kaiser CA. Nitrogen regulation in Saccharomyces cerevisiae Gene. 2002;290(1–2):1–18.

    Article  CAS  PubMed  Google Scholar 

  45. Dempsey WB. Metabolism of α-aminoisobutyric acid by soil bacteria. J Bacteriol. 1969;97(1):182–5.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  46. Kellis M, Patterson N, Endrizzi M, Birren B, Lander ES. Sequencing and comparison of yeast species to identify genes and regulatory elements. Nature. 2003;423(6937):241–54.

    Article  CAS  PubMed  Google Scholar 

  47. Bricmont PA, Daugherty JR, Cooper TG. The DAL81 gene product is required for induced expression of two differently regulated nitrogen catabolic genes in Saccharomyces cerevisiae Mol Cell Biol. 1991;11(2):1161–6.

    CAS  PubMed  PubMed Central  Google Scholar 

  48. Sylvain MA, Liang XB, Hellauer K, Turcotte B. Yeast zinc cluster proteins Dal81 and Uga3 cooperate by targeting common coactivators for transcriptional activation of γ-aminobutyrate responsive genes. Genetics. 2011;188(3):523–34.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  49. Davis MA, Small AJ, Kourambas S, Hynes MJ. The tamA gene of Aspergillus nidulans contains a putative zinc cluster motif which is not required for gene function. J Bacteriol. 1996;178(11):3406–9.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  50. Tornow J, Zeng X, Gao W, Santangelo GM. GCR1, a transcriptional activator in Saccharomyces cerevisiae, complexes with RAP1 and can function without its DNA binding domain. EMBO J. 1993;12(6):2431–7.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  51. Hahn S, Young ET. Transcriptional regulation in Saccharomyces cerevisiae: Transcription factor regulation and function, mechanisms of initiation, and roles of activators and coactivators. Genetics. 2011;189(3):705–36.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  52. Iraqui I, Vissers S, André B, Urrestarazu A. Transcriptional induction by aromatic amino acids in Saccharomyces cerevisiae Mol Cell Biol. 1999;19(5):3360–71.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  53. Martens JA, Wu PYJ, Winston F. Regulation of an intergenic transcript controls adjacent gene transcription in Saccharomyces cerevisiae Genes Dev. 2005;19(22):2695–704.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  54. Scott S, Abul-Hamd AT, Cooper TG. Roles of the Dal82p domains in allophanate/oxalurate-dependent gene expression in Saccharomyces cerevisiae J Biol Chem. 2000;275(40):30886–93.

    Article  CAS  PubMed  Google Scholar 

  55. Coelho MA, Gonçalves C, Sampaio JP, Gonçalves P. Extensive intra-kingdom horizontal gene transfer converging on a fungal fructose transporter gene. PLoS Genet. 2013;9(6):e1003587.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  56. Yamaguchi H, Kodama H, Osada S, Kato F, Jelokhani-Niaraki M, Kondo M. Effect of α, α-dialkyl amino acids on the protease resistance of peptides. Biosci Biotechnol Biochem. 2003;67(10):2269–72.

    Article  CAS  PubMed  Google Scholar 

  57. Degenkolb T, Gräfenhan T, Berg A, Nirenberg HI, Gams W, Brückner H. Peptaibiomics: screening for polypeptide antibiotics (peptaibiotics) from plant-protective Trichoderma species. Chem Biodivers. 2006;3(6):593–610.

    Article  CAS  PubMed  Google Scholar 

  58. Marik T, Tyagi C, Balázs D, Urbán P, Szepesi Á, Bakacsy L, et al. Structural diversity and bioactivities of peptaibol compounds from the longibrachiatum clade of the filamentous fungal genus Trichoderma. Front Microbiol. 2019;10.

  59. Scannell DR, Zill OA, Rokas A, Payen C, Dunham MJ, Eisen MB, et al. The awesome power of yeast evolutionary genetics: New genome sequences and strain resources for the Saccharomyces sensu stricto genus. G3 Genes Genomes Genet. 2011;1(1):11–25.

    CAS  Google Scholar 

  60. Macías LG, Morard M, Toft C, Barrio E. Comparative genomics between Saccharomyces kudriavzevii and S. cerevisiae applied to identify mechanisms involved in adaptation. Front Genet. 2019;10:187.

    Article  PubMed  PubMed Central  Google Scholar 

  61. Altschul SF, Gish W, Miller W, Myers EW, Lipman DJ. Basic local alignment search tool. J Mol Biol. 1990;215(3):403–10.

    Article  CAS  PubMed  Google Scholar 

  62. Brickwedde A, Brouwers N, van den Broek M, Gallego Murillo JS, Fraiture JL, Pronk JT, et al. Structural, physiological and regulatory analysis of maltose transporter genes in Saccharomyces eubayanus CBS 12357T. Front Microbiol. 2018;9.

  63. Quevillon E, Silventoinen V, Pillai S, Harte N, Mulder N, Apweiler R, et al. InterProScan: protein domains identifier. Nucleic Acids Res. 2005;33:W116–20.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  64. Gietz RD, Schiestl RH. Frozen competent yeast cells that can be transformed with high efficiency using the LiAc/SS carrier DNA/PEG method. Nat Protoc. 2007;2(1):1–4.

    Article  CAS  PubMed  Google Scholar 

  65. Baudin A, Ozier-kalogeropoulos O, Denouel A, Lacroute F, Cullin C. A simple and efficient method for direct gene deletion in Saccharomyces cerevisiae Nucleic Acids Res. 1993;21(14):3329–30.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  66. Goldstein AL, McCusker JH. Three new dominant drug resistance cassettes for gene disruption in Saccharomyces cerevisiae Yeast. 1999;15(14):1541–53.

    Article  CAS  PubMed  Google Scholar 

  67. Güldener U, Heck S, Fiedler T, Beinhauer J, Hegemann JH. A new efficient gene disruption cassette for repeated use in budding yeast. Nucleic Acids Res. 1996;24(13):2519–24.

    Article  PubMed  PubMed Central  Google Scholar 

  68. Stovicek V, Holkenbrink C, Borodina I. CRISPR/Cas system for yeast genome engineering: advances and applications. FEMS Yeast Res. 2017;17(5).

  69. Doench JG, Hartenian E, Graham DB, Tothova Z, Hegde M, Smith I, et al. Rational design of highly active sgRNAs for CRISPR-Cas9-mediated gene inactivation. Nat Biotechnol. 2014;32(12):1262–7.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  70. Generoso WC, Gottardi M, Oreb M, Boles E. Simplified CRISPR-Cas genome editing for Saccharomyces cerevisiae J Microbiol Methods. 2016;127:203–5.

    Article  CAS  PubMed  Google Scholar 

  71. Dicarlo JE, Norville JE, Mali P, Rios X, Aach J, Church GM. Genome engineering in Saccharomyces cerevisiae using CRISPR-Cas systems. Nucleic Acids Res. 2013;41(7):4336–43.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  72. Pronk JT. Auxotrophic yeast strains in fundamental and applied research. Appl Environ Microbiol. 2002;68(5):2095–100.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  73. Kahm M, Hasenbrink G, Lichtenberg-Fraté H, Ludwig J, Kschischo M. grofit: fitting biological growth curves with R. J Stat Softw. 2010;33(7):1–21.

    Article  Google Scholar 

  74. Kushnirov VV. Rapid and reliable protein extraction from yeast. Yeast. 2000;16(9):857–60.

    Article  CAS  PubMed  Google Scholar 

  75. Redruello B, Ladero V, del Rio B, Fernández M, Martin MC, Alvarez MA. A UHPLC method for the simultaneous analysis of biogenic amines, amino acids and ammonium ions in beer. Food Chem. 2017;217:117–24.

    Article  CAS  PubMed  Google Scholar 

  76. Edgar RC. MUSCLE: multiple sequence alignment with high accuracy and high throughput. Nucleic Acids Res. 2004;32(5):1792–7.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  77. Tamura K, Stecher G, Kumar S. MEGA11: molecular evolutionary genetics analysis version 11. Mol Biol Evol. 2021;38(7):3022–7.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  78. Darriba D, Taboada GL, Doallo R, Posada D. ProtTest 3: Fast selection of best-fit models of protein evolution. Bioinformatics. 2011;27(8):1164–5.

    Article  CAS  PubMed  Google Scholar 

  79. Le SQ, Gascuel O. An improved general amino acid replacement matrix. Mol Biol Evol. 2008;25(7):1307–20.

    Article  CAS  PubMed  Google Scholar 

  80. Jones DT, Taylor WR, Thornton JM. The rapid generation of mutation data matrices. Bioinformatics. 1992;8(3):275–82.

    Article  CAS  Google Scholar 

  81. Schmidt HA, Strimmer K, Vingron M, von Haeseler A. TREE-PUZZLE: maximum likelihood phylogenetic analysis using quartets and parallel computing. Bioinformatics. 2002;18:502–4.

    Article  CAS  PubMed  Google Scholar 

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We thank the members of our group for helping us with the bioinformatics analyses and the group led by Dr. Paloma Manzanares for methodological assistance for the protein activity validation.


This study has received funding from the European Union’s Horizon 2020 research and innovation program under the Marie Sklodowska-Curie grant agreement number 764364, Aromagenesis, from the Spanish government and EU ERDF-FEDER projects RTI2018-093744-B-C31 and RTI2018-093744-B-C32 to AQ and EB, respectively, and from the Center of Excellence Accreditation “Severo Ochoa” program of the Spanish government, ref. CEX2021-001189-S/MCIN/AEI/ 10.13039/501100011033.

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Authors and Affiliations



Author contributions were as follows: SMT—methodology, experiment design, investigation, validation, visualization, data analysis, and writing-original draft. LGM—genome assembly and annotation, database management, homologous gene search, and phylogenetic analysis. RPT—supervision, writing—review, and editing. ND—experimental assistance, investigation. PM—methodological assistance and experiment design. AQ—conceptualization, writing review, funding acquisition, project administration, and supervision. EB—conceptualization, writing review and editing, homologous gene search, phylogenetic analysis curation, funding acquisition, and supervision. All authors read and approved the final manuscript.

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Correspondence to Eladio Barrio.

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Supplementary Information

Additional file 1: Table S1.

Source of the SaccharomycesAQ assemblies used for the blastn search. This table contains the source of the Saccharomyces genome sequences where the cluster containing the putative genes FT, AT, and AAP were present or not found.


Additional file 2.


Additional file 3.


Additional file 4.


Additional file 5.


Additional file 6.


Additional file 7.


Additional file 8.

Additional file 9: Table S2.

Primers for AQ2901 and IFO1802 DGD1 alleles cloning used in this study. Table S3. Escherichia coli strains used in this study. Table S4. HPLC program for AIB quantification. Table S6. Primers for the DGD2 zinc finger motif sequencing.

Additional file 10: Table S5.

Genomic screening of the gene cluster in budding yeast species. Green: orthologous gene present. Red: orthologous gene not found.


Additional file 11.


Additional file 12.


Additional file 13.

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Tapia, S.M., Macías, L.G., Pérez-Torrado, R. et al. A novel aminotransferase gene and its regulator acquired in Saccharomyces by a horizontal gene transfer event. BMC Biol 21, 102 (2023).

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  • Saccharomyces
  • HGT
  • Dialkylglycine decarboxylase
  • DGD1
  • AIB