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A single Gal4-like transcription factor activates the Crabtree effect in Komagataella phaffii

Abstract

The Crabtree phenotype defines whether a yeast can perform simultaneous respiration and fermentation under aerobic conditions at high growth rates. It provides Crabtree positive yeasts an evolutionary advantage of consuming glucose faster and producing ethanol to outcompete other microorganisms in sugar rich environments. While a number of genetic events are associated with the emergence of the Crabtree effect, its evolution remains unresolved. Here we show that overexpression of a single Gal4-like transcription factor is sufficient to convert Crabtree-negative Komagataella phaffii (Pichia pastoris) into a Crabtree positive yeast. Upregulation of the glycolytic genes and a significant increase in glucose uptake rate due to the overexpression of the Gal4-like transcription factor leads to an overflow metabolism, triggering both short-term and long-term Crabtree phenotypes. This indicates that a single genetic perturbation leading to overexpression of one gene may have been sufficient as the first molecular event towards respiro-fermentative metabolism in the course of yeast evolution.

Introduction

The fermentative activity of yeast has been used to make bread and fermented beverages by mankind since its early settlement. Thus the physiological capabilities of yeast are directly linked to human development and culture. These processes depend fundamentally on the respiro-fermentative phenotype also called the Crabtree effect of some yeast species, most prominently baker’s yeast (Saccharomyces cerevisiae).

A similar phenomenon as the Crabtree effect can be observed in cancer cells which have high glycolytic rates and lactic acid fermentation, termed the Warburg effect1. The Crabtree effect of S. cerevisiae is seen as a unicellular model to study the genetic and metabolic control of the Warburg effect2,3,4,5,6.

Being a fundamental feature of yeast metabolism, the Crabtree phenotype defines whether a yeast can perform simultaneous respiration and fermentation under aerobic conditions at high growth rates. Crabtree-positive (respiro-fermenting) yeasts, such as S. cerevisiae, Vanderwaltozyma polyspora, Torulaspora franciscae, Lachancea waltii, and Lachancea kluyveri (syn. Saccharomyces kluyveri) can exhibit alcoholic fermentation in the presence of oxygen until glucose reaches low concentrations7,8. Nevertheless, rather few yeasts show this phenotype. In most cases, glucose uptake and glycolysis are strictly regulated to match the TCA cycle capacity, so the exclusive use of respiration leads to full oxidation of glucose to CO2 and water with maximum energy yield under aerobic conditions. These yeasts, such as Yarrowia lipolytica, Candida albicans, Eremothecium coryli, and Komagataella phaffii (syn. Pichia pastoris) are defined as Crabtree negative (respiring) yeasts8.

It is assumed that the Crabtree phenotype first evolved 125–150 million years ago (mya) in the Saccharomyces lineage around the same time as flowering plants which provided a sugar-rich niche for yeasts. The occurrence of the overflow metabolism was the first step in the evolution of aerobic fermentation in yeast8,9,10,11. There are a number of genetic events that contributed to the emergence of the Crabtree effect in the evolutionary history: whole genome duplication12,13, horizontal transfer of the URA1 gene14, rewiring of the transcriptional network15,16, loss of respiratory complex I17, and duplication of hexose transporter genes18. Besides this evolutionary development in the Saccharomyces lineage, the Crabtree-positive phenotype has evolved several times independently in yeasts16,19.

Crabtree-positive yeasts have several genes for low-affinity hexose transporters enabling high transport rates at high sugar concentration. On the contrary, Crabtree-negative yeasts usually have only one or two low-affinity HXT genes but several high-affinity transporters20. Accordingly, lower specific glucose uptake rates in Crabtree-negative yeasts prevent the overflow metabolism that causes reduced biomass yield and ethanol production at high glucose concentrations under aerobic conditions in Crabtree-positive yeasts.

K. phaffii is a canonical Crabtree-negative yeast and able to ferment in oxygen-limited conditions21. It possesses two high affinity and two low-affinity glucose transporters similar to other respiratory yeasts such as Kluyveromyces lactis, Hansenula polymorpha, and Scheffersomyces stipitis20. Consequently, the specific glucose uptake rate at maximum specific growth rate in K. phaffii is 8-fold lower22 in comparison to respiro-fermentative S. cerevisiae23.

Here we show that glycolysis and fermentation are controlled by a single transcription factor (TF) in K. phaffii, and that its overexpression is sufficient to convert the Crabtree phenotype, indicating that this regulatory switch in phenotype could have easily occurred during evolution. We characterize the Crabtree phenotype of mutant K. phaffii strains and compare it to other Crabtree negative and positive yeasts. Additionally, we investigate transcriptomes and central metabolic fluxes to characterize the physiological responses to overexpression and deletion of the transcription factor. As we show that K. phaffii switches to a respiro-fermentative phenotype by altered expression of a single gene, it will be important to investigate in future if K. phaffii might be a better model for the Warburg effect than S. cerevisiae.

Results

A single TF enhances glucose uptake and ethanol production

Recently, we identified a transcription factor as an activator of the glyceraldehyde 3-phosphate dehydrogenase promoter24 which has sequence similarity to S. cerevisiae Gal4. Putative Gal4 specific transcription factor (TF) binding sites were found in all glycolytic promoters of K. phaffii, and overexpression of the GAL4-like TF gene led to growth defects in a K. phaffii strain when grown in glucose surplus. These results prompted us to dissect the role of this transcription factor on central carbon metabolism of K. phaffii as it is obvious that it is not involved in galactose metabolism since K. phaffii cannot metabolize galactose.

Overexpression (OE) of this TF changed specific rates of growth, glucose consumption, and ethanol production markedly, as well as biomass and ethanol yields (Table 1 and Supplementary Figure 1), and led to a 1.7-fold higher glucose uptake rate and a 10-fold elevated ethanol yield in shake flask cultivations. Together with the increased ethanol production, the overexpression strain exhibited a diauxic growth profile typical for Crabtree-positive yeasts (Fig. 1). The biomass yield on glucose (YX/S) of the overexpression strain was 1.9-fold lower at the expense of ethanol formation. In contrast, no ethanol was produced by the deletion strain and the specific glucose uptake rate was 2.2-fold lower compared to the control strain, further underlining the role of the Gal4-like transcription factor in the regulation of glucose metabolism. Based on its obvious role in glycolysis and fermentation we decided to allocate a novel name to this transcription factor and suggest CRA1, referring to its impact on the Crabtree phenotype of K. phaffii.

Table 1 Overexpression or deletion of the GAL4-like TF gene changes the phenotype of K. phaffii
Fig. 1
figure1

GAL4-like overexpression strains consume glucose faster and produce ethanol. Biomass dry weight (green), glucose consumption (magenta) and ethanol production (orange) profiles of the control strain (dashed line) and GAL4-like overexpression mutants (solid line). Values of 3 different independent transformants of the control (empty circles) and 4 overexpressing the GAL4-like TF (filled circles) are shown

A glucose pulse triggers fermentation in the CRA1 OE strain

To verify that the CRA1 overexpression strain is a true Crabtree-positive yeast we investigated its short- and long-term Crabtree phenotype. The short-term Crabtree effect is defined as the response of a non-fermenting culture at steady-state to an excess glucose pulse. As described by Hagman and coworkers25, control and CRA1 overexpression strains were grown in steady-state chemostat at a dilution rate D = 0.1 h−1, followed by a glucose pulse of CGlucose = 9–11 g L−1. We also performed the same experiments with S. cerevisiae and Kluyveromyces marxianus as internal controls, and verified that our data is comparable to Hagman et al25. During the first hour after the glucose pulse biomass of the control strain increased, while it remained unchanged in the cultures of the CRA1 overexpression strain. Glucose consumption profiles demonstrated the differences in short-term Crabtree phenotype between the control and CRA1 overexpression strains. While they had a similar specific glucose consumption rate during the steady-state cultivation, it was 1.2-fold higher in the overexpression strain within the first 20 min after the glucose pulse and then decreased (Fig. 2a and Supplementary Table 1). Similarly, higher specific glucose uptake rates were achieved in comparison to other Crabtree negative and positive yeasts except Vanderwaltozyma polyspora (Fig. 2a). In addition, the ethanol concentration produced by the K. phaffii CRA1 overexpression strain increased to 0.23 g L−1 after the first 20 min which is comparable to other short-term Crabtree-positive yeasts and reached 0.35 g L−1 during the first hour after the glucose pulse which is a typical behavior for fermenting yeasts (Fig. 2aand Supplementary Table 1). The specific ethanol production rate of the overexpression strain was in the range of other Crabtree-positive yeasts.

Fig. 2
figure2

The CRA1 overexpression strain exhibits a short-term Crabtree phenotype. K. phaffii strains were grown in chemostat at D = 0.1 h−1 in steady state, followed by a glucose pulse of 9-11 g L−1. Data of K. phaffii control, overexpression strain, Saccharomyces cerevisiae CEN.PK113-5D and Kluyveromyces marxianus CBS712 (indicated with an asterisk) are shaded dark. The data of other yeast species were retrieved from Hagman et al.25 and shaded light. They comprise the Crabtree positive species (above the dashed line) Vanderwaltozyma polyspora, S. cerevisiae, Lachancea waltii, Lachancea kluyveri, Torulaspora franciscae, Kluyveromyces lactis, and the Crabtree negative species (below the dashed line) Debaryomyces vanrijiae, Eremothecium coryli, K. marxianus and P. pastoris (syn. Komagataella sp.). a Comparison of specific glucose consumption (blue) and ethanol formation (red) rates. The specific glucose uptake rate of the CRA1 overexpression strain was higher compared to the control strain and other Crabtree-negative yeasts. Ethanol production by the CRA1 overexpression strain was comparable to other short-term Crabtree-positive yeasts, while the control strain did not produce ethanol, same as the other Crabtree-negative yeasts. b O2 uptake (orange) and CO2 evolution rates (green) among other yeasts based on their short-term Crabtree effect. Calculated CO2 evolution rate values for the CRA1 overexpression strain were in the range of other short-term Crabtree-positive yeasts (see ref. 25). Mean values of the duplicate bioreactor cultivations for the control and overexpression K. phaffii strains are presented. Error bars represent the standard deviation (±)

CO2 production of yeast has two primary sources: respiration and fermentation. After the glucose pulse, the K. phaffii CRA1 overexpression mutant reached higher CO2 evolution rates (CER) compared to the control strain, as 2 moles of CO2 per mole O2 are produced during fermentation different to respiration in which 1 mole O2 consumption corresponds to 1 mole CO2. Following the glucose pulse, CER of K. phaffii CRA1 overexpression mutants reached 4.53 mmol g−1 h−1 which was 1.7-fold higher compared to the control strain as well as other Crabtree-negative yeasts (Fig. 2b). These findings fit well to the data from other Crabtree-positive yeasts where CER varied from 3.2–7.0 mmol g−1 h−1 25 (Fig. 2b and Supplementary Table 1).

The long-term Crabtree effect is triggered by CRA1 OE

The long-term Crabtree effect is defined as the ability of a yeast strain to ferment glucose to ethanol under aerobic conditions in a glucose-limited chemostat. The critical dilution rate (Dcrit) is defined as the strain-specific threshold value at which the yeast metabolism switches from respiratory state to respiro-fermentative state where ethanol formation starts. In other words, above Dcrit, ethanol is produced as the glucose flux exceeds the critical value towards the TCA cycle. A Crabtree-negative yeast, however, grows in a respiratory state and is washed out without ethanol formation when the maximum dilution rate (Dmax) is exceeded. We conducted chemostat cultivations to determine the critical dilution rate threshold for the K. phaffii CRA1 overexpression strain (Fig. 3 and Supplementary Table 2).

Fig. 3
figure3

The long-term Crabtree effect is triggered by overexpression of CRA1. The control strain exhibited a fully respiratory metabolism and was washed out after Dmax = 0.4 h−1 (upper panel). The metabolic activity of the CRA1 overexpression strain, however, shifted from respiratory metabolism to respiro-fermentative metabolism and started to produce ethanol when Dcrit = 0.27 h−1 was achieved (lower panel). Above Dcrit glucose consumption rates increased sharply while biomass concentrations dropped. Mean values of biomass dry weight concentration (squares), specific glucose consumption (circles) and specific ethanol production rates (triangles) of the control and CRA1 overexpression strain at different dilution rates during the chemostats are given (chemostats were performed in duplicates). Gray and black lines show the dilution rates of the biological replicates at which the cells were washed out

With the increase in dilution rate (D), the specific glucose uptake rates increased accordingly, and similar specific glucose uptake rates were obtained for the control and the CRA1 overexpression strains until D = 0.25 h−1. The control strain could grow in fully respiratory state without any ethanol formation until the dilution rate reached Dmax = 0.4 h−1 and was washed out when the dilution rate was further increased to 0.45 h−1. However, the CRA1 overexpression mutant displayed a clear long-term Crabtree phenotype above D = 0.25 h−1: the cell concentration decreased, and ethanol production began at Dcrit = 0.27 h−1. When compared to the control strain, a 1.7-fold higher specific glucose consumption rate was achieved by the overexpression strain at the critical dilution rate (Dcrit = 0.27 h−1) indicating a higher glycolytic flux. Accordingly, ethanol production started, showing that a fraction of metabolic activity shifted from respiratory metabolism to respiro-fermentative metabolism. When the dilution rate was further increased to D = 0.32 h−1, the cells were washed out and could not reach a new steady-state showing that Dcrit = Dmax = 0.27 h−1 for the CRA1 overexpression strain.

Comparison of several yeast species based on their specific glucose consumption rates, respiratory quotients, specific ethanol production rates, CER, oxygen uptake rates (OUR), and maximum specific growth rates revealed that there is a universal cut-off value for glucose consumption rates which is around 10–15 C-mmol g−1 h−1 8. This is the cut-off value where Crabtree-positive yeasts exhibit an imbalanced catabolic and anabolic metabolism, due to a loss of coordination between glucose consumption and growth. This results in an overflow in carbon metabolism, leading to ethanol production. Indeed, the K. phaffii CRA1 overexpression strain started to produce ethanol when qS exceeded 15.8 C-mmol g−1 h−1 (Fig. 3 and Supplementary Table 2) as opposed to the control strain where the balance could be preserved between glucose consumption rate and carbon flux towards catabolic and anabolic pathways at even higher growth rates.

The CRA1 OE strain classifies as Crabtree-positive yeast

Crabtree phenotype defines whether a yeast can perform simultaneous respiration and fermentation under aerobic conditions. However, not every Crabtree-positive yeast shows this phenotype in the same range. Hagman and coworkers26 classified 11 different yeast genera (including 55 different strains of 34 species) into 4 groups, based on their ethanol and biomass yields on glucose, specific glucose consumption rates and specific growth rates in a batch culture. Among these, group 1 includes the Crabtree-negative yeasts and groups 2–4 include Crabtree-positive yeasts. We used this classification as an indicator to rate the Crabtree phenotype of the CRA1 overexpression strain among other yeasts and divided yeasts into 2 different groups: group 1 includes the Crabtree-negative yeasts (including 15 different strains of 8 species) and group 2 (including 40 different strains of 26 species from groups 2–426) contains the Crabtree-positive yeasts (having a Crabtree phenotype in different ranges) (Fig. 4). The K. phaffii control strain fell into Group 1 with other Crabtree-negative yeasts. The CRA1 overexpression strain, however, was classified as a Crabtree-positive yeast in Group 2.

Fig. 4
figure4

The CRA1 overexpression strain classifies as a Crabtree-positive yeast. Classification of yeasts based on a ethanol yield, b biomass yield, and c specific glucose consumption rate reveals that the control strain, K. phaffii (blue), belongs to Group 1 with other Crabtree-negative yeasts (Eremothecium and Kluyveromyces genera, see ref. 26). K. phaffii CRA1 overexpression strain (red), however, is classified as a Crabtree-positive yeast with other positive yeast species (Lachancea, Torulaspora, Zygotorulaspora, Vandervaltozyma, Tetrapisispora, Saccharomyces, Kazachstania, Naumovozyma, and Nakaseomyces genera). Values of the duplicate experiments for the control and overexpression K. phaffii strains are presented. The box plots are based on the data of ref. 25. The box spans the interquartile range (second and third quartile), middle line represents the median value and whiskers show the minimum and maximum values

Upregulation of glycolytic genes causes metabolic imbalance

For an in-depth analysis of the effect of the Cra1 TF on regulation of the glycolytic pathway, we conducted RNASeq and 13C labeled metabolic flux analysis (MFA) (Fig. 5). Transcript levels of glycolytic (HXK1, PGI1, PFK1, PFK2, FBA1-1, TDH3, ENO1, GPM1, CDC19) and fermentative genes (PDC1, ADH2) were upregulated in the CRA1 overexpression strain compared to the control strain while the genes responsible for the TCA cycle (CIT1, ACO1, IDP1, KGD2, FUM1, MDH1, MDH3) remained unchanged. In agreement with the RNASeq data, the glycolytic flux was more than twofold higher in the CRA1 overexpression strain. The split ratio (%) at the glucose-6-phosphate node was 85/15 (± 1.5) (glycolysis/pentose phosphate pathway) in the CRA1 overexpression strain, compared to 44/56 (± 0.1) in the control strain. Around the pyruvate node, the ratio (%) between fermentation and respiration was 68/32 (± 13) (ethanol/acetyl CoA) in the overexpression strain compared to 17/83 (± 21) in the control. Comparing specific carbon fluxes, a decrease of pentose phosphate pathway and TCA cycle fluxes contributed to the 10-fold increase of specific fermentation flux. This finding is in agreement with the situation in S. cerevisiae, where higher glycolytic fluxes cause a decrease in the TCA fluxes8,27,28. The increase of specific NADH production in lower glycolysis between control and overexpression strain of 4.7 mmol g−1 h−1 balances well with the increased specific NADH consumption in ethanol formation of 5.4 mmol g−1 h−1, and thus restores the redox balance in the CRA1 overexpression strain through respiratory-fermentative metabolism. These data further support the hypothesis that a single gene controls the development of a Crabtree positive strain by upregulating all relevant glycolytic and fermentative genes.

Fig. 5
figure5

13C metabolic flux analysis and RNASeq explain the overflow metabolism. Glycolysis and fermentation correlate with pathway gene upregulation in the CRA1 overexpression strain. Absolute specific flux rates per carbon atom (C-mmol g−1h −1) of control, CRA1 overexpression and Δcra1 strains are given from top to bottom. For reversible fluxes, only net fluxes are shown. Gene names of the corresponding reactions are colored green for transcriptionally upregulated, and black for unregulated genes in the CRA1 overexpression strain compared to the control. The insert table displays the respective log2 fold changes and adjusted p-values. NA means data did not meet filter criteria for p-value calculation (see Methods). Mean values of triplicate experiments for the control, overexpression and knock-out K. phaffii strains are presented. ± represents the standard deviation. Values of each reaction refer to the total number of carbon atoms involved in this reaction. For clarity of the figure, fluxes to CO2 are not shown

In addition to the glycolytic and fermentative pathway genes mentioned above, several other genes were also found to be upregulated in the CRA1 overexpression strain. Of these, the genes responsible for thiamine biosynthesis (THI20, THI4, THI11) were upregulated in the CRA1 overexpression strain (and downregulated in the Δcra1 strain) compared to the control. THI7 was downregulated in the Δcra1 strain in comparison to the control in addition to the downregulated thiamine genes mentioned above. As thiamine is required for several enzymes of the central carbon metabolism like pyruvate decarboxylase, pyruvate dehydrogenase or transketolase, increased transcript levels of thiamine biosynthesis genes were expected. In S. cerevisiae, disruption of THI2 and THI3 was shown to impair pyruvate decarboxylase activity, enhancing pyruvate production and decreasing ethanol formation29. In this yeast, PDC and thiamine biosynthesis genes are linked by a common transcriptional activator, Pdc230. Up to now, no homolog of PDC2 was identified in K. phaffii, but it is interesting that a convergent co-regulation by a Gal4-like TF is present.

Discussion

When we analyzed the promoter sequences of the glycolytic genes in K. phaffii, putative binding sites of a Gal4-like TF were found24. K. phaffii does not possess a galactose metabolism31, therefore it is obvious that this TF is not involved in galactose utilization. As the previous gene designation (GAL4) was solely based on its sequence similarity to the ortholog in S. cerevisiae, we attributed a new short name to the gene PP7435_Chr1-1522 as CRA1 to avoid any confusion related to the different roles of this gene in K. phaffii and S. cerevisiae, respectively. K. phaffii is a canonical Crabtree-negative yeast and its glucose uptake capacity is limited13. However, the overexpression of CRA1 resulted in a significant increase in glucose uptake rate and ethanol yield compared to the control strain (Fig. 1 and Table 1). Given the fact that the specific glucose uptake rate of a Δcra1 strain was 2.2-fold lower compared to the control strain, it appears that CRA1 has a regulatory role in glucose metabolism of K. phaffii. Indeed, the CRA1 overexpression strain was classified as a Crabtree-positive yeast contrary to the control strain (Fig. 4). Both short- and long-term Crabtree phenotypes were triggered in the CRA1 overexpression strain (Figs 23) indicating an overflow of the glycolytic flux due to the overexpression of CRA1. Upregulation of the glycolytic genes and an increase in glucose uptake rate resulted in higher glycolytic flux towards lower glycolysis, obviously causing an imbalance between respiration and biomass formation (Fig. 5). This higher and imbalanced glycolytic flux then caused an overflow metabolism which led to an increased flux through the fermentative pathway, i.e. ethanol production which is a typical phenotype for the majority of the respiro-fermenting yeasts including species from SaccharomycesKluyveromyces, Lachancea, Torulaspora, Zygotorulaspora8.

Several evolutionary mechanisms have been proposed to understand how the Crabtree phenotype emerged. The Crabtree effect arose several times in yeast evolution16,19. In the Saccharomyces lineage, the extent of the Crabtree effect in each species relates to its position in the phylogenetic tree9. A whole genome duplication (WGD) event approximately 100 mya ago13 and a global rewiring of the rapid growth elements11,13 that changed the regulation of genes associated with respiration and rapid growth, are the major evolutionary steps that contributed to the ability of ethanol production. It has been suggested that the Crabtree effect originated approximately 125 mya with the horizontal transfer of the URA1 gene which enabled yeasts to grow anaerobically after the loss of respiratory chain complex I14,17. However, our data suggest that deregulation of a single transcription factor can lead to the invention of the Crabtree effect, without the requirement of anaerobic growth or loss of respiratory chain complex I. This was also suggested as a possible scenario by Dashko and coworkers9 based on the data of Hagman et al.26 They suggest that the initial evolutionary driving force in sugar-rich environments may have been connected to regular exposure to oxygen-limited niches, so that yeasts developed strengthened glycolytic and fermentation pathways for anaerobic growth. This may have been the later basis for the development of aerobic fermentation. Previously we showed that in hypoxic conditions the fermentative pathway is switched on in K. phaffii, and glycolysis is upregulated21. This means, K. phaffii ferments with higher glycolytic flux and higher glucose uptake rates in oxygen limitation, but not in aerobic conditions. By overexpression of CRA1, the joint regulation of glycolysis and fermentation leads to the Crabtree positive phenotype, without the need of any other mutation such as the change of URA1 or the loss of respiratory complex I. This suggests that aerobic fermentation may have occurred very early in yeast evolution, even before anaerobic growth was fully established.

Dashko and coworkers9 also pointed out the role of hexose transporters in glucose utilization and argue that multiplication of hexose transporters could be one of the molecular backgrounds for the increased glucose consumption ability. Interestingly, the hexose transporter genes were not upregulated by CRA1 overexpression indicating that the increase in the glucose uptake rate is driven by the enhanced glycolytic flux rather than the upregulation of hexose transporter genes. We calculated the kinetic parameters, Km and Vmax, and a two-tailed Student’s t-test showed that there is no statistically significant difference (p-value = 0.68) between the Km values of the control (Km = 14.1 ± 3.8 mM) and the CRA1 overexpression strain (Km = 12.8 ± 3.3 mM). Vmax values, however, differed significantly (control: 0.85 g g−1 h−1, CRA1 overexpression: 1.49 g−1 h−1 h, p-value = 0.002).

According to Martchenko et al.32 Gal4 was recruited (together with Mig1) late in ascomycete yeast evolution to regulate the Leloir pathway for galactose utilization. In yeasts that originate from ancestors prior to this transition, such as C. albicans, Debaryomyces hansenii, or Schizosaccharomyces pombe, the Leloir pathway genes are controlled by Cph1. K. lactis and Naumovozyma castellii (syn. Saccharomyces castellii) appear to mark the transition, having both Gal4 and Mig1 as well as Cph1 binding sites in the Gal gene promoters, while later in evolution, Saccharomyces species have lost Cph1 binding sites. Deletion of the GAL4-like gene in C. albicans indicated that it is involved in regulation of glycolysis32,33. GAL4 of S. cerevisiae is regulated at the transcriptional level and by the accessory proteins Gal80 and Gal3. K. phaffii and other Crabtree-negative yeasts do not possess homologs of Gal80 and Gal334. In K. phaffii the CRA1 gene is transcriptionally upregulated in glucose surplus35 and under severe glucose limitation, when compared to limited but reasonably good supply with glucose like in the chemostat36,37.

We analyzed glycolytic and GAL gene promoters of S. cerevisiae, Kazachstania naganishii, N. castellii, Zygosaccharomyces rouxii, L. kluyveri, Eremothecium gossypii (syn. Ashbya gossypii), K. lactis, C. albicans, Sugiyamaella lignohabitans, D. hansenii, Y. lipolytica, and Ogataea parapolymorpha for the presence of Gal4 binding sites (Supplementary Table 3). A high number of Gal4 binding sites (around 20–30 in total) in promoters of glycolytic genes were found in K. phaffii, E. gossypii, D. hansenii, K. naganishii, S. lignohabitans, O. parapolymorpha, and C. albicans, while the other yeast genomes contain lower numbers of binding sites in glycolytic gene promoters. K. naganashii and Z. rouxii apparently mark transitions with similar, rather high numbers of binding sites in both pathways. With these two exceptions, a high number of Gal4 binding sites in galactose utilization gene promoters correlates with a decreased number in glycolytic promoters, supporting the general hypothesis that during evolution Gal4 switched its function from a generalist TF regulating the central carbon metabolism to a specialist TF responsible for the galactose metabolism34. We overexpressed the native CRA1 homolog (annotated as GAL4) in S. lignohabitans to test whether it acts as a generalist TF on the central carbon metabolism in this yeast as well. Indeed, overexpression of GAL4 resulted in a 1.3-fold increase in specific glucose uptake rate and a 1.5-fold increase in specific glycerol production rate, respectively (Supplementary Table 4). Glycerol is a by-product of the central carbon metabolism, produced to sustain the redox balance similar to ethanol. These data support the hypothesis that the Gal4 ortholog acts as a generalist TF of glucose metabolism in Crabtree-negative yeasts.

Up to now, the evolution of the Crabtree phenotype has been linked to several complex genetic and metabolic changes i.e. whole genome duplication, loss of respiratory complex I, and rewiring of the transcriptional network. Here we show that a single transcription factor controls glycolysis and fermentation of the Crabtree-negative yeast K. phaffii. Its overexpression is sufficient to convert K. phaffii to a Crabtree-positive yeast, indicating that a single mutation may have been sufficient as a first evolutionary event towards respiro-fermentative metabolism. Apart from shedding new light on the evolution of the Crabtree effect in yeasts, this novel K. phaffii strain may serve as a better model to study the Warburg effect of cancer cells.

Methods

Strains

All strains were derived from the parental strain Komagataella phaffii CBS7435. CRA1 overexpression strains were constructed by using GoldenPiCS38. The Δcra1 strain was obtained by the split marker cassette method39. In part of the strains the eGFP gene (under control of the glyceraldehyde-3-phosphate dehydrogenase promoter (PGAP)) was used as a reporter of CRA1 based induction of glycolytic genes. These strains were used in RNASeq and 13C metabolic flux analysis. In all the transformations, at least 3 random transformants were selected as biological replicates for further shake flask experiments to minimize the risk of accidental spurious mutations that could cause phenotypic changes. We also used two different background strains to overexpress CRA1 (Table 2) which resulted in the same phenotypic changes. One representative transformant was used for RNASeq and 13C metabolic flux analysis. Two different biological replicates for each strain were used in chemostat cultures.

Table 2 K. phaffii strains used in the study

A BLAST analysis was performed to identify the putative GAL4 ortholog of S. lignohabitans (NCBI RefSeq Accession Number: XP_018737608.1 [https://www.ncbi.nlm.nih.gov/protein/XP_018737608.1/]). After PCR amplification from S. lignohabitans strain CBS10342 the gene was cloned into an integration vector under control of PGAP of S. lignohabitans and transformed into the same strain40.

Shake flask cultivations

All shake flask experiments were performed in 200 mL wide neck shake flasks with 20 mL M2 medium containing (g L−1) 5 glucose, 3.15 (NH4)2HPO4; 0.49 MgSO4.7H2O; 0.8 KCl; 0.0268 CaCl2.2H2O; 22 citric acid monohydrate; 1.47 mL PTM; 2 mL biotin (0.2 g L−1). Cells grown in YP medium for 24–26 h were washed and transferred into M2 medium. Samples were collected during the exponential growth phase for the characterization of the strains (in duplicates), calculation of the kinetic parameters (Vmax and Km) of the glucose transporters (in triplicates), 13C metabolic flux analysis (in triplicates) and RNASeq analysis (in triplicates).

Chemostat cultivations for long-term and short-term Crabtree effect

All chemostat cultivations were performed in duplicate in DASGIP (Jülich, Germany) bioreactors with a working volume of 1 L. pH was controlled at 5.00 with 12.5% ammonia solution. Dissolved oxygen concentration was kept above 30% with a constant airflow of 16 L h−1. One mL cryostock of K. phaffii strains were inoculated into 100 mL of YPG medium (g L−1: 10 yeast extract, 20 soy-peptone, 20 glycerol) including 25 μg L−1 Zeocin as preculture and incubated at 25 °C and 180 rpm for approximately 24 h. This culture was inoculated to the bioreactor with an OD600 of 0.3 to initiate batch cultivation. Batch medium included (g L−1) 2 citrate monohydrate, 12.6 (NH4)2HPO4, 0.5 MgSO4.7H2O, 0.9 KCl, 0.022 CaCl2.2H2O, 4.6 mL PTM, 2 ml biotin (0.2 g L−1). 10 g L−1 and 7.2 g L−1 glycerol was added to the batch medium for the investigation of long-term and short-term Crabtree effects, respectively. PTM stock solution contained (g L−1) 6.0 CuSO4∙5H2O, 0.08 NaI, 3.36 MnSO4∙H2O, 0.2 Na2MoO4∙2H2O, 0.02 H3BO3, 0.82 CoCl2, 20.0 ZnCl2, 65.0 FeSO4∙7H2O and 5.0 mL H2SO4 (95%–98%). Following the batch end, chemostat cultivation was started.

Investigation of the short-term Crabtree effect of the K. phaffii control and overexpression strains was performed in 700 mL medium at 25 °C with a similar experimental design made by Hagman and coworkers25. Cells were grown in chemostat cultivation at D = 0.1 h−1 at fully respiring conditions. After five residence times until steady state was achieved, a glucose pulse was applied to the cultures to a final concentration of 9–11 g L−1 (t = 0 min) and samples were taken every 20 min. Chemostat medium contained (g L−1) 0.36 citrate monohydrate, 7.92 glucose monohydrate, 3.13 (NH4)2HPO4, 0.14 MgSO4.7H2O, 0.36 KCl, 0.005 CaCl2.2H2O, 0.35 ml PTM, 0.29 biotin (0.2 g L−1). Batch and chemostat cultivations for S. cerevisiae CEN.PK113-5D and K. marxianus CBS712 were performed in the same chemostat medium but supplemented with vitamin solutions: (mg L−1) 0.04 biotin, 0.72 calcium pantothenate, 0.72 nicotinic acid, 18.0 myo-inositol, 0.72 thiamine HCl, 0.72 pyridoxine, 0.14 para-aminobenzoic acid. Additionally, uracil with a concentration of 54 mg L−1 was used for cultivation of uracil auxotrophic S. cerevisiae CEN.PK113-5D.

Evaluation of the long-term Crabtree effect of the strains was carried out in 350 mL medium at 30 °C in fully respiring conditions. Chemostat cultivation was started with a dilution rate (D) 0.1 h−1 and increased incrementally until ethanol formation set in and increased further until cells were washed out. Samples were collected for each dilution rate after five residence times when steady state was reached. Chemostat medium contained (g L−1) 0.5 citrate monohydrate, 11.0 glucose monohydrate, 4.35 (NH4)2HPO4, 0.2 MgSO4.7H2O, 0.5 KCl, 0.007 CaCl2.2H2O, 0.48 mL PTM, 0.4 mL biotin (0.2 g L−1).

Analysis of bioreactor samples

For determination of dry cell weight (DCW), culture broth was centrifuged; pellets were washed with distilled water and dried for 24 h at 100 °C in preweighed glass tubes. Harvested supernatants were used for measurement of extracellular metabolites, and their concentrations were quantified by HPLC analysis41. Specific growth rates, glucose uptake rates and metabolite secretion rates were calculated based on the HPLC measurements. CO2 evolution rates (CER) and O2 utilization rates (OUR) were calculated by using an off-gas analyzer.

13C metabolic flux analysis

Culture broth (corresponding approximately to 15–20 mg total dry biomass) was mixed with 60% (v/v) cold methanol (< −20 °C) for quenching and filtered immediately42. Metabolites were extracted using boiling ethanol extraction43.

13C labeling patterns of intracellular metabolites were analyzed by GC-QTOFMS44. Specific growth, glucose uptake and metabolite secretion rates were calculated during the exponential growth phase. Biomass composition of the control, overexpression and knock-out strains were assumed to be similar to those determined previously by Carnicer and coworkers45.

The stoichiometric model (Supplementary Table 5) used for the calculation of intracellular fluxes was based on a previously published model of K. phaffii central carbon metabolism46. OpenFLUX with default settings was used for flux calculation applying the gradient based search algorithm for sensitivity analysis by a Monte Carlo algorithm47. Mass distribution values and sensitivity analysis results are provided in Supplementary Table 6. All calculations were done with MATLAB (R2013a, The MathWorks, Inc., Natick, Massachusetts, USA).

RNASeq analysis

Pellets from the samples collected during the exponential growth phase were resuspended in 1 mL TRI Reagent (Sigma, USA). Cells were disrupted by glass beads using a ribolyser (MP Biomedicals, USA) for 40 s at 5.5 ms-1. RNA was extracted by chloroform and precipitated with isopropanol. After washing twice with 75% ethanol, RNA was dissolved in nuclease-free water. After DNase treatment (Invitrogen, USA), concentration of RNA was measured by Nanodrop and quality of the samples was verified with the Agilent Bioanalyzer 2100 using the RNA 6000 Nano Assay kit (Agilent Technologies, California, USA). RNA sequencing was performed with poly(A)-enriched mRNAs at Vienna Biocenter Core Facilities GmbH (AT). cDNA libraries were constructed from these poly(A)-enriched mRNAs and sequenced by Illumina HiSeq v4.

Processing of the RNASeq data

The resulting unsorted and unaligned BAM files where sorted with samtools sort v1.5, followed by conversion and splitting into paired-end FASTQ files by using picard tools v2.17.3-3-g3bf7fdc-SNAPSHOT SamToFastq (https://broadinstitute.github.io/picard/). Subsequently the files where trimmed and quality checked using TrimGalore v0.4.2 (http://www.bioinformatics.babraham.ac.uk/projects/trim_galore/) with default parameters. As preparation for the count quantification a transcript index was created using the latest K. phaffii CBS7435 annotation (FR839628.1, FR839629.1, FR839630.1, FR839631.1, FR839632.1; October 2016) and the kallisto v0.43.048 subprogram index. Annotations of the genes were based on the recent curation by Valli et al.49 which included 5325 open reading frames and 16 mitochondrial genes. Afterwards the read count for each sample was determined using kallisto subprogram quant50. For differential expression analysis51 with R (http://www.R-project.org/) the packages tximport and tximportData52, readr (https://CRAN.R-project.org/package=readr) and DESeq2 (https://rdrr.io/bioc/DESeq2)53,54,55 were used for each comparison. Based on the determination of the differential expression by using DESeq2 some fold-change or p-values are not displayed (represented as NA). This result can occur in three cases: Firstly, if all samples of a row have zero counts, secondly, if a sample denotes an extreme count outlier (detected by Cook’s distance) and finally a sample row is excluded by automated filtering for having a low mean normalized count54. Visualization of the expression analysis results was also carried out with R. Cutoff criteria were a minimum fold-change of 2 and an adjusted p-value lower than 0.05 (Supplementary Data 1).

Characterization of glucose transport kinetics

Vmax and Km values of the glucose transporters of the control and CRA1 overexpression strains were determined based on Michaelis-Menten kinetics. Specific glucose consumption rates were calculated by using M2 medium with different initial glucose concentrations, i.e. 2.5, 5.0, 10.0, and 20 g L−1. Samples were collected during the exponential growth phase. Residual glucose and biomass concentrations were measured to calculate the specific glucose uptake rates. A Lineweaver-Burk plot was used to dissect the Michaelis-Menten equation and determine the kinetic parameters.

Promoter sequence analysis

Putative Gal4 transcription factor binding sites in the promoter sequences of the glycolytic and galactose metabolism genes of 13 yeast species were analyzed by MatInspector release 8.4.1 within the Genomatix Suite56 by using the Matrix Family Library Version 11.0 for fungi. Default settings were left unchanged and matching scores higher than 0.75 were considered. Only positions with a predicted binding site on both DNA strands were considered as true matches. 1000 bp upstream of the genes were considered as the promoter sequences and sequences were retrieved from Genome Resources for Yeast Chromosomes (GRYC), National Center for Biotechnology Information (NCBI) and www.pichiagenome.org.

Reporting Summary

Further information on research design is available in the Nature Research Reporting Summary linked to this article.

Data availability

Raw data of the RNASeq analysis was deposited to the NCBI Gene Expression Omnibus (GEO) repository under accession number [GSE110624]. All other data are available upon reasonable request from the corresponding author (DM).

Additional information

Publisher’s note: Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

References

  1. 1.

    Warburg, O., B., Wind, F. & Negelein, N. The metabolism of tumors in the body. J. Gen. Physiol. 309, 397–519 (1927).

  2. 2.

    Peeters, K. et al. Fructose-1,6-bisphosphate couples glycolytic flux to activation of Ras. Nat. Commun. 8, 922 (2017).

  3. 3.

    Shulman, R. G. & Rothman, D. L. Homeostasis and the glycogen shunt explains aerobic ethanol production in yeast. Proc. Natl Acad. Sci. USA 112, 10902–10907 (2015).

  4. 4.

    Tosato, V. et al. Warburg effect and translocation-induced genomic instability: two yeast models for cancer cells. Front. Oncol. 2, 212 (2013).

  5. 5.

    Diaz-Ruiz, R., Rigoulet, M. & Devin, A. The Warburg and Crabtree effects: On the origin of cancer cell energy metabolism and of yeast glucose repression. Biochim. Biophys. Acta 1807, 568–576 (2011).

  6. 6.

    Diaz-Ruiz, R., Uribe-Carvajal, S., Devin, A. & Rigoulet, M. Tumor cell energy metabolism and its common features with yeast metabolism. Biochim. Biophys. Acta 1796, 252–265 (2009).

  7. 7.

    De Deken, R. The Crabtree effects: a regulatory system in yeast. J. Gen. Microbiol. 44, 149–156 (1966).

  8. 8.

    Hagman, A. & Piškur, J. A study on the fundamental mechanism and the evolutionary driving forces behind aerobic fermentation in yeast. PLoS ONE 10, e0116942 (2015).

  9. 9.

    Dashko, S., Zhou, N., Compagno, C. & Piškur, J. Why, when, and how did yeast evolve alcoholic fermentation? Fems. Yeast. Res. 14, 826–832 (2014).

  10. 10.

    Pfeiffer, T. & Morley, A. An evolutionary perspective on the Crabtree effect. Front. Mol. Biosci. 1, 17 (2014).

  11. 11.

    Piškur, J., Rozpedowska, E., Polakova, S., Merico, A. & Compagno, C. How did Saccharomyces evolve to become a good brewer? Trends Genet. 22, 183–186 (2006).

  12. 12.

    Conant, G. C. & Wolfe, K. H. Increased glycolytic flux as an outcome of whole-genome duplication in yeast. Mol. Syst. Biol. 3, 129 (2007).

  13. 13.

    Wolfe, K. H. & Shields, D. C. Molecular evidence for an ancient duplication of the entire yeast genome. Nature 387, 708–713 (1997).

  14. 14.

    Gojković, Z. et al. Horizontal gene transfer promoted evolution of the ability to propagate under anaerobic conditions in yeasts. Mol. Genet. Genom. 271, 387–393 (2004).

  15. 15.

    Ihmels, J. et al. Rewiring of the yeast transcriptional network through the evolution of motif usage. Science 309, 938–940 (2005).

  16. 16.

    Rozpędowska, E. et al. Parallel evolution of the make-accumulate-consume strategy in Saccharomyces and Dekkera yeasts. Nat. Commun. 2, 302 (2011).

  17. 17.

    Marcet-Houben, M., Marceddu, G. & Gabaldán, T. Phylogenomics of the oxidative phosphorylation in fungi reveals extensive gene duplication followed by functional divergence. BMC Evol. Biol. 9, 295 (2009).

  18. 18.

    Lin, Z. & Li, W. H. Expansion of hexose transporter genes was associated with the evolution of aerobic fermentation in yeasts. Mol. Biol. Evol. 28, 131–142 (2011).

  19. 19.

    Lin, Z. & Li, W. H. The Evolution of aerobic fermentation in Schizosaccharomyces pombe was associated with regulatory reprogramming but not nucleosome reorganization. Mol. Biol. Evol. 28, 1407–1413 (2011).

  20. 20.

    Mattanovich, D. et al. Genome, secretome and glucose transport highlight unique features of the protein production host Pichia pastoris. Microb. Cell. Fact. 8, 29 (2009).

  21. 21.

    Baumann, K. et al. The impact of oxygen on the transcriptome of recombinant S. cerevisiae and P. pastoris - a comparative analysis. BMC Genom. 12, 218 (2011).

  22. 22.

    Maurer, M., Kühleitner, M., Gasser, B. & Mattanovich, D. Versatile modeling and optimization of fed batch processes for the production of secreted heterologous proteins with Pichia pastoris. Microb. Cell. Fact. 5, 37 (2006).

  23. 23.

    Otterstedt, K. et al. Switching the mode of metabolism in the yeast Saccharomyces cerevisiae. EMBO Rep. 5, 532–537 (2004).

  24. 24.

    Ata, Ö., Prielhofer, R., Gasser, B., Mattanovich, D. & Çalık, P. Transcriptional engineering of the glyceraldehyde-3-phosphate dehydrogenase promoter for improved heterologous protein production in Pichia pastoris. Biotechnol. Bioeng. 114, 2319–2327 (2017).

  25. 25.

    Hagman, A., Säll, T. & Piškur, J. Analysis of the yeast short-term Crabtree effect and its origin. Febs. J. 281, 4805–4814 (2014).

  26. 26.

    Hagman, A., Säll, T., Compagno, C. & Piškur, J. Yeast ‘Make-Accumulate-Consume’ Life Strategy Evolved as a Multi-Step Process That Predates the Whole Genome Duplication. PLoS One 8, e68734 (2013).

  27. 27.

    Frick, O. & Wittmann, C. Characterization of the metabolic shift between oxidative and fermentative growth in Saccharomyces cerevisiae by comparative 13C flux analysis. Microb. Cell. Fact. 4, 30 (2005).

  28. 28.

    Vemuri, G. N., Eiteman, M. A., McEwen, J. E., Olsson, L. & Nielsen, J. Increasing NADH oxidation reduces overflow metabolism in Saccharomyces cerevisiae. Proc. Natl. Acad. Sci. USA 104, 2402–2407 (2007).

  29. 29.

    Xu, G., Hua, Q., Duan, N., Liu, L. & Chen, J. Regulation of thiamine synthesis in Saccharomyces cerevisiae for improved pyruvate production. Yeast 29, 209–217 (2012).

  30. 30.

    Nosaka, K. Recent progress in understanding thiamin biosynthesis and its genetic regulation in Saccharomyces cerevisiae. Appl. Microbiol. Biotechnol. 72, 30–40 (2006).

  31. 31.

    Kurtzman, C. P. Description of Komagataella phaffii sp. nov. and the transfer of Pichia pseudopastoris to the methylotrophic yeast genus Komagataella. Int. J. Syst. Evol. Microbiol. 55, 973–976 (2005).

  32. 32.

    Martchenko, M., Levitin, A., Hogues, H., Nantel, A. & Whiteway, M. Transcriptional rewiring of fungal galactose-metabolism circuitry. Curr. Biol. 17, 1007–1013 (2007).

  33. 33.

    Askew, C. et al. Transcriptional regulation of carbohydrate metabolism in the human pathogen Candida albicans. PLoS. Pathog. 5, e1000612 (2009).

  34. 34.

    Choudhury, B. I. & Whiteway, M. Evolutionary transition of GAL regulatory circuit from generalist to specialist function in ascomycetes. Trends Microbiol. 26, 692–702 (2018).

  35. 35.

    Prielhofer, R. et al. Pichia pastoris regulates its gene-specific response to different carbon sources at the transcriptional, rather than the translational, level. BMC Genom. 16, 167 (2015).

  36. 36.

    Rebnegger, C. et al. In Pichia pastoris, growth rate regulates protein synthesis and secretion, mating and stress response. Biotechnol. J. 9, 511–525 (2014).

  37. 37.

    Rebnegger, C. et al. Pichia pastoris exhibits high viability and a low maintenance energy requirement at near-zero specific growth rates. Appl. Environ. Microbiol. 82, 4570–4583 (2016).

  38. 38.

    Prielhofer, R. et al. GoldenPiCS: a Golden Gate-derived modular cloning system for applied synthetic biology in the yeast Pichia pastoris. BMC Syst. Biol. 11, 123 (2017).

  39. 39.

    Heiss, S., Maurer, M., Hahn, R., Mattanovich, D. & Gasser, B. Identification and deletion of the major secreted protein of Pichia pastoris. Appl. Microbiol. Biotechnol. 97, 1241–1249 (2013).

  40. 40.

    Bellasio, M. et al. Complete genome sequence and transcriptome regulation of the pentose utilizing yeast Sugiyamaella lignohabitans. Fems. Yeast. Res. 16, fow037 (2016).

  41. 41.

    Pflügl, S., Marx, H., Mattanovich, D. & Sauer, M. 1,3-Propanediol production from glycerol with Lactobacillus diolivorans. Bioresour. Technol. 119, 133–140 (2012).

  42. 42.

    Russmayer, H. et al. Metabolomics sampling of Pichia pastoris revisited: rapid filtration prevents metabolite loss during quenching. Fems. Yeast. Res. 15, fov049 (2015).

  43. 43.

    Neubauer, S. et al. U 13C cell extract of Pichia pastoris - a powerful tool for evaluation of sample preparation in metabolomics. J. Sep. Sci. 35, 3091–3105 (2012).

  44. 44.

    Mairinger, T. et al. Gas chromatography-quadrupole time-of-flight mass spectrometry-based determination of isotopologue and tandem mass isotopomer fractions of primary metabolites for 13C-metabolic flux analysis. Anal. Chem. 87, 11792–11802 (2015).

  45. 45.

    Carnicer, M. et al. Macromolecular and elemental composition analysis and extracellular metabolite balances of Pichia pastoris growing at different oxygen levels. Microb. Cell. Fact. 8, 65 (2009).

  46. 46.

    Baumann, K. et al. A multi-level study of recombinant Pichia pastoris in different oxygen conditions. BMC Syst. Biol. 4, 141 (2010).

  47. 47.

    Quek, L. E., Wittmann, C., Nielsen, L. K. & Krömer, J. O. OpenFLUX: Efficient modelling software for 13C-based metabolic flux analysis. Microb. Cell. Fact. 8, 25 (2009).

  48. 48.

    Bray, N. L., Pimentel, H., Melsted, P. & Pachter, L. Near-optimal probabilistic RNA-seq quantification. Nat. Biotechnol. 34, 525–527 (2016).

  49. 49.

    Valli, M. et al. Curation of the genome annotation of Pichia pastoris (Komagataella phaffii) CBS7435 from gene level to protein function. Fems. Yeast. Res. 16, fow051 (2016).

  50. 50.

    Bray, N. L., Pimentel, H. Melsted, P. & Pachter L. Near-optimal RNA-Seq quantification. Preprint at: https://arxiv.org/abs/1505.02710 (2015).

  51. 51.

    Love, M. I., Anders, S., Kim, V. & Huber, W. RNA-Seq workflow: gene-level exploratory analysis and differential expression. F1000Res. 4, 1070 (2015).

  52. 52.

    Soneson, C., Love, M. I. & Robinson, M. D. Differential analyses for RNA-seq: transcript-level estimates improve gene-level inferences. F1000Res. 4, 1521 (2015).

  53. 53.

    Huber, W. et al. Orchestrating high-throughput genomic analysis with Bioconductor. Nat. Methods 12, 115–121 (2015).

  54. 54.

    Gentleman, R. et al. Bioconductor: open software development for computational biology and bioinformatics. Genome Biol. 5, R80 (2004).

  55. 55.

    Love, M. I., Huber, W. & Anders, S. Moderated estimation of fold change and dispersion for RNA-seq data with DESeq2. Genome Biol. 15, 550 (2014).

  56. 56.

    Cartharius, K. et al. MatInspector and beyond: Promoter analysis based on transcription factor binding sites. Bioinformatics 21, 2933–2942 (2005).

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Acknowledgements

We thank Hannes Rußmayer for his support in sample preparation for GC-QTOFMS analysis of 13C labeled metabolites. A special thank is due to the late Prof. Jure Piškur for sharing his knowledge and enthusiasm on yeast metabolism and evolution of fermentation. ÖA was awarded scholarships by the Scientific and Technical Research Council of Turkey (TÜBİTAK-BIDEB) and the Austrian Agency for International Cooperation in Education and Research (OeAD), financed by the Austrian Federal Ministry of Science, Research and Economy (BMWFW) (grant no. ICM-2017-06356). This work has been partly supported by the Austrian Federal Ministry for Digital and Economic Affairs (BMDW), the Federal Ministry of Traffic, Innovation and Technology (bmvit), the Styrian Business Promotion Agency SFG, the Standortagentur Tirol, the Government of Lower Austria and ZIT – Technology Agency of the City of Vienna through the COMET-Funding Program managed by the Austrian Research Promotion Agency FFG, and by the Christian Doppler Research Association, the Austrian Federal Ministry for Digital and Economic Affairs (BMDW) and the National Foundation for Research, Technology and Development (CR). Vienna Business Agency and EQ BOKU VIBT GmbH are acknowledged for providing mass spectrometry and bioreactor instrumentation.

Author information

ÖA contributed to the design of the study and performed the shake flask and bioreactor cultivations, promoter motif analysis, samplings for RNASeq and 13C labeled metabolic flux experiments, data analysis and interpretation, and drafted the manuscript. CR performed the bioreactor cultivations. NET performed the RNASeq data processing and investigated the statistical significance of the results. MV helped with the K. phaffii genome annotation and interpretation of the RNASeq analysis results. TM and SH performed the GC-MS experiments for 13C labeled metabolites. MGS contributed to the design of the 13C labeled metabolic flux analysis experiment, helped with the interpretation of the results and revised the manuscript. PÇ contributed to study design and experimental planning. DM designed the study, contributed to the data analysis, drafted and revised the manuscript. All authors read and approved the final manuscript.

Competing interests

The authors declare no competing interests.

Correspondence to Diethard Mattanovich.

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