Open Access

Transcriptional activator Cat8 is involved in regulation of xylose alcoholic fermentation in the thermotolerant yeast Ogataea (Hansenula) polymorpha

  • Justyna Ruchala1,
  • Olena O. Kurylenko2,
  • Nitnipa Soontorngun3,
  • Kostyantyn V. Dmytruk2 and
  • Andriy A. Sibirny1, 2Email author
Microbial Cell Factories201716:36

https://doi.org/10.1186/s12934-017-0652-6

Received: 29 November 2016

Accepted: 23 February 2017

Published: 28 February 2017

Abstract

Background

Efficient xylose alcoholic fermentation is one of the key to a successful lignocellulosic ethanol production. However, regulation of this process in the native xylose-fermenting yeasts is poorly understood. In this work, we paid attention to the transcriptional factor Cat8 and its possible role in xylose alcoholic fermentation in Ogataea (Hansenula) polymorpha. In Saccharomyces cerevisiae, organism, which does not metabolize xylose, gene CAT8 encodes a Zn-cluster transcriptional activator necessary for expression of genes involved in gluconeogenesis, respiration, glyoxylic cycle and ethanol utilization. Xylose is a carbon source that could be fermented to ethanol and simultaneously could be used in gluconeogenesis for hexose synthesis. This potentially suggests involvement of CAT8 in xylose metabolism.

Results

Here, the role of CAT8 homolog in the natural xylose-fermenting thermotolerant yeast O. polymorpha was characterized. The CAT8 ortholog was identified in O. polymorpha genome and deleted both in the wild-type strain and in advanced ethanol producer from xylose. Constructed cat8Δ strain isolated from wild strain showed diminished growth on glycerol, ethanol and xylose as well as diminished respiration on the last substrate. At the same time, cat8Δ mutant isolated from the best available O. polymorpha ethanol producer showed only visible defect in growth on ethanol. CAT8 deletant was characterized by activated transcription of genes XYL3, DAS1 and RPE1 and slight increase in the activity of several enzymes involved in xylose metabolism and alcoholic fermentation. Ethanol production from xylose in cat8Δ mutants in the background of wild-type strain and the best available ethanol producer from xylose increased for 50 and 30%, respectively. The maximal titer of ethanol during xylose fermentation was 12.5 g ethanol/L at 45 °C. Deletion of CAT8 did not change ethanol production from glucose. Gene CAT8 was also overexpressed under control of the strong constitutive promoter GAP of glyceraldehyde-3-phosphate dehydrogenase. Corresponding strains showed drop in ethanol production in xylose medium whereas glucose alcoholic fermentation remained unchanged. Available data suggest on specific role of Cat8 in xylose alcoholic fermentation.

Conclusions

The CAT8 gene is one of the first identified genes specifically involved in regulation of xylose alcoholic fermentation in the natural xylose-fermenting yeast O. polymorpha.

Keywords

Transcriptional activator Xylose High-temperature alcoholic fermentation Yeast Ogataea (Hansenula) polymorpha

Background

Fermentation is the largest field of industrial biotechnology. In 2014, near 95 billion liters of ethanol were produced [1]. Currently, most of industrial ethanol is produced from starch and sucrose (1st generation ethanol), however, due to limited feedstock abundance, further increase in fuel ethanol production will depend on development of feasible technology of alcoholic fermentation from lignocellulose (2nd generation ethanol). One of the most important goals in the development of such technology is construction of strains capable of efficient fermentation of lignocellulosic pentoses, especially xylose, which constitutes about 30% of all sugars in lignocellulosic hydrolyzates [2, 3]. It would also be useful to carry out fermentation of xylose and other lignocellulosic sugars under elevated temperatures (around 50 °C), which would allow optimal activities of cellulases and hemicellulases necessary for the process known as Simultaneous Saccharification and Fermentation (SSF) [4]. In such a process, free sugars liberated by enzymatic hydrolysis do not exert product inhibition on hydrolyzing enzymes, since they are simultaneously converted to ethanol by thermotolerant microorganisms in the same vessel. Very few yeast organisms are capable of high-temperature alcoholic fermentation, namely Kluyveromyces marxianus [5] and Ogataea (Hansenula) polymorpha [6, 7]. Current work focuses on O. polymorpha which is the most thermotolerant yeast species known to date, with maximal growth and fermentation temperatures of 50 °C or even higher [8, 9]. It has been reported that O. polymorpha produces ethanol from glucose, cellobiose, glycerol and xylose at elevated temperatures [7, 10], however, ethanol yield and productivity from xylose by the wild-type strains is very low [11]. O. polymorpha can also produce ethanol directly from starch and xylan after expression of heterologous genes encoding corresponding hydrolytic enzymes [12]. Several methods of metabolic engineering, both original and those developed for other yeast species, were successfully used for improvements of ethanol synthesis from xylose in O. polymorpha. They include heterologous expression of bacterial xylose isomerases and overexpression of native xylulokinase [13] and, alternatively, overexpression of engineered xylose reductase with decreased affinity to NADPH as well as native xylitol dehydrogenase and xylulokinase [14] and overexpression of pyruvate decarboxylase in the strain unable to utilize ethanol as sole carbon source [15]. Combination of metabolic engineering (overexpression of engineered xylose reductase and native xylitol dehydrogenase and xylulokinase) with classical selection approaches (selection for strains unable to utilize ethanol as sole carbon source and resistant to glycolysis inhibitor 3-bromopyruvate), allowed isolation of strains that accumulate 15–20 times more ethanol from xylose relative to the wild-type strain, i.e. around 10 g ethanol/L at 45 °C [16]. While mutation(s) causing resistance to 3-bromopyruvate in the ethanol overproducing strain remain to be identified, we have recently mapped a corresponding mutation in the strain with the wild-type background and showed that it disrupted an autophagy-related gene ATG13. This mutation led to a 50% increase in ethanol production from xylose [17]; Dmytruk, Sibirny, in preparation]. Still, the achieved yield and productivity of ethanol synthesis from xylose are lower than that described for engineered Saccharomyces cerevisiae and several native xylose-fermenting yeasts (which however are mesophilic and therefore could not be useful for the SSF process). Further possible increase in ethanol synthesis by O. polymorpha from xylose is hampered due to absence of the knowledge on regulation of xylose metabolism and fermentation. Therefore, it is important to identify the corresponding genes and, depending on their functions, activate or repress them. Described functions of a transcription factor Cat8 (encoded by CAT8 gene) in activating multiple metabolic processes in S. cerevisiae, mostly gluconeogenesis and ethanol utilization [18, 19], led us to hypothesize that it might also be involved in regulation of xylose metabolism in O. polymorpha. One of the reasons that just CAT8 was selected among multiple genes coding for transcription factors involved in carbon metabolism [20] was that knock out of CAT8 activated glucose alcoholic fermentation in S. cerevisiae [21] and non-conventional yeast Pichia guilliermondii [22]. Xylose is a unique carbon source as it could be fermented to ethanol, similarly to glucose, and simultaneously it has to be converted to glucose and other hexoses, mostly in pentose phosphate pathway though partial contribution of gluconeogenesis in hexose synthesis from xylose cannot be neglected. We hypothesized that for these reasons the mutants of O. polymorpha with knock out of the ortholog of CAT8 gene will have impairments in xylose respiration and gluconeogenesis, so the flux of this sugar will be activated instead into fermentation direction.

Roles of CAT8 gene in regulation of cell metabolism are quite well understood in S. cerevisiae. It encodes a Zn-cluster transcriptional activator necessary for expression of genes involved in gluconeogenesis, ethanol utilization and diauxic shift from fermentation to respiration [18, 19]. Strains with deletion of CAT8 show defects in growth on ethanol, glycerol and other gluconeogenic substrates whereas disaccharides are utilized normally. Mechanistically, Cat8 exerts transcriptional activation of its target genes by binding to carbon source-responsive elements in their regulatory promoters [20, 23]. However, the limited data available on the functions of CAT8 in non-Saccharomyces yeasts show differences in functions of the corresponding orthologs. Thus, Kluyveromyces lactis mutant defective in CAT8 showed defects in ethanol utilization, whereas growth on glycerol was normal [24]. cat8Δ mutant of Candida albicans normally utilized all carbon substrates tested [25], whereas growth patterns of the mutant with knock out of CAT8 in Pichia guilliermondii were not assayed at all [22]. Role of CAT8 in regulation of xylose metabolism is poorly understood. Transcriptome analysis of the natural xylose-metabolizing yeast O. polymorpha did not find changes in CAT8 expression between xylose- and glucose-containing media [26]. In recombinant S. cerevisiae capable of xylose metabolism, xylose caused only weak repression of CAT8 relative to glucose suggesting xylose growing cells are in between totally repressed and derepressed state regarding catabolite repression [27].

To test our hypothesis on the role of Cat8 transcription factor in xylose fermentation, we have isolated CAT8 knock-out mutants in O. polymorpha on either wild-type or ethanol overproducing (from xylose) strain [16]. We also overexpressed CAT8. In favor of our hypothesis, we found that strains with deletions of CAT8Δ accumulate more ethanol during xylose fermentation, while ethanol production from glucose was not changed. Mutant O. polymorpha cat8 isolated from the advanced ethanol producer accumulated up to 12.5 g ethanol/L at 45 °C, which is the highest ethanol titer for high-temperature xylose fermentation. Inversely, strain of O. polymorpha with overexpression of CAT8 accumulated less ethanol relative to the parental wild-type strain.

Results

Isolation and growth characteristics of cat8Δ mutants

We decided to delete the O. polymorpha CAT8 ortholog in both wild-type strain and the best ethanol producer (BEP) from xylose [16] and to study the properties of the resulted deletants. In particular, we focused on growth patterns, respiration, activity of some enzymes, expression of selected genes and ethanol production in xylose and glucose media. Genome of O. polymorpha strain NCYC495 is sequenced and is publicly available [28]. It contains single ortholog of S. cerevisiae gene CAT8, which shows 31% identity and 53% similarity to CAT8 gene of S. cerevisiae. To knock it out in O. polymorpha, a deletion cassette was constructed, which contained natNT2 gene conferring resistance to nourseothricin as a selection marker, flanked with non-coding regions of the CAT8 gene ortholog (see “Methods” section; Additional file 1A). Homologous recombination resulted in isolation of the cat8Δ strain. In total, near 1000 nourseothricin-resistant transformants were analyzed and 9 of them appeared to be cat8Δ mutants. Our attempts to isolate cat8Δ on the background of strain BEP were unsuccessful. In total, we analyzed near 2000 transformants and invariably without success. It is known that the selection marker has strong impact on the efficiency of homologous recombination [29]. Therefore, we decided to construct a deletion cassette using a selection marker gene hphNT1, conferring resistance to hygromycin (see “Methods” section; Additional file 1B). In this case, 10 CAT8 knock out mutants were identified among 400 analyzed hygromycin-resistant transformants.

The isolated cat8Δ mutants on the background of the wild-type and BEP strains were assayed for growth, biochemical and physiological characteristics. Growth of these mutants was analyzed in YNB solid and liquid media supplemented with different carbon sources and compared with that of the corresponding parental strain. It was found that isolated mutants normally grew in media with glucose, whereas growth of cat8Δ mutant isolated from wild-type strain on glycerol and ethanol was retarded but not totally abolished. Growth of BEP cat8Δ was very similar to that of BEP in glycerol containing medium, while BEP cat8Δ was unable to growth in ethanol, unlike to BEP (Additional file 2). It is remarkable that growth of cat8Δ strain isolated from the wild-type strain on xylose was also partially retarded, whereas no significant difference in growth on xylose was observed between BEP and BEP cat8Δ strains. However, the BEP strain much better grows on xylose relative to the wild-type strain apparently due to overexpression of genes XYL1, XYL2 and XYL3 involved in primary xylose metabolism [16] (Fig. 1; Additional file 2). It has to be pointed out that ethanol overproducing strain BEP poorly grows on ethanol [16], whereas its derivative BEP cat8Δ mutant did not grow on this substrate at all. We suggest that function of CAT8 in O. polymorpha is similar to that in S. cerevisiae as corresponding deletants grow poorly on ethanol and glycerol.
Fig. 1

Growth of the strains with deletion (cat8∆) or overexpression of CAT8 gene (CAT8*) on different carbon sources (glucose, xylose, glycerol, ethanol) as compared to the parental strains

Isolation and growth characteristics of the strains with overexpression of CAT8

Transformants of O. polymorpha wild-type strain, which express CAT8 under control of the strong constitutive GAP promoter of glyceraldehyde-3-phosphate dehydrogenase gene, were isolated (WT CAT8). Overexpression of CAT8 was proved by qRT-PCR. It was found that indeed, the analyzed strain with CAT8 gene under GAP promoter showed increase in CAT8 expression for 2.65 times (Additional file 3). It was found that WT CAT8 did not differ from the wild-type strain regarding growth on the tested substrates: glucose, xylose, glycerol and ethanol (Fig. 1).

Respiration, enzymatic profiles and transcription of selected genes in the isolated mutants

More detailed physiological, biochemical and genetic analyses were carried out on constructed deletion mutants cat8Δ and BEP cat8Δ. To reveal the role of CAT8 gene in the metabolism of O. polymorpha, cell respiration of cat8Δ cells in glucose- and xylose-containing media was studied. It was found that cells of both cat8Δ and BEP cat8Δ strains showed up to 40% decrease in respiration with xylose as a substrate. Respiration of cat8Δ but not that of BEP cat8Δ cells also was decreased using glucose as a substrate (Table 1). These data confirm our suggestion on the similar role of CAT8 in O. polymorpha and S. cerevisiae. The observed small increase in glucose respiration of BEP cat8Δ cells apparently depends on unidentified mutations introduced in BEP strain during its selection [16]. In the following experiments, we analyzed specific activities of several enzymes involved in xylose metabolism and ethanol synthesis in cells cultivated in xylose medium. It was found that deletion of CAT8 led to moderate increase in specific activities of most of the analyzed enzymes involved in xylose metabolism and alcoholic fermentation: xylose reductase, xylulokinase, transketolase, pyruvate decarboxylase and alcohol dehydrogenase. Activity of fructose-1,6-bisphosphatase in cat8Δ mutants was slightly increased whereas xylitol dehydrogenase activity was, inversely, decreased as compared to that of the parental strains (Table 2). Cat8 protein is apparently involved in the regulation of the corresponding gene expression. To test this hypothesis, transcription profiles of several potentially involved genes were studied using quantitative reverse-transcription PCR (qRT-PCR). It was found that cat8Δ mutant isolated from the wild-type strain cultivated in xylose medium showed higher level of XYL3, DAS1 and RPE1 mRNAs whereas expression of the other analyzed genes (XYL1, XYL2, PDC1, TKL1, TAL1, TAL2, FBP1, PCK1) was quite similar as compared to that of the wild-type strain (Table 3). Strain BEP cat8Δ revealed increased expression of RPE1, decreased expression of XYL1, XYL2 and DAS1 while the expression of other tested genes possessed minor fluctuations relative to that of BEP strain on xylose containing medium (Table 3). Expression of RPE1 was increased for both deletion mutants to infer this gene as a promising target for overexpression, aiming to increase performance of xylose alcoholic fermentation. We also assayed the relative expression of the studied genes between O. polymorpha wild-type strain NCYC495 and the BEP strain as it was not done previously [16]. It showed a substantial enhancement of the expression of genes involved in xylose metabolism in ethanol overproducing strain with especially high increase in expression of RPE1 gene (Table 3). We speculate that this was achieved by metabolic engineering of the first steps of xylose metabolism but also possibly as a result of classical selection [16].
Table 1

Respiration activity of analyzed O. polymorpha strains

Strain

Respiration (nanomoles of O2 consumed per minute per mg of cells at 30 °C)

Glucose as substrate

Xylose as substrate

WT

11.81 ± 0.52

11.35 ± 0.56

cat8Δ

8.49 ± 0.07

7.08 ± 0.14

BEP

11.87 ± 0.59

17.17 ± 0.86

BEP cat8Δ

13.98 ± 0.70

10.53 ± 0.02

Determinations were performed in distilled air-saturated water with the concentration of cells 0.5 g/L of dry weight and started by addition of 1% carbon substrate (glucose or xylose). The respiratory rate was expressed as nanomoles of O2 consumed per minute per mg of cells (dry weight)

Table 2

Specific activities of XR (xylose reductase), XDH (xylitol dehydrogenase), XK (xylulokinase), ADH (alcohol dehydrogenase), PDC (pyruvate decarboxylase), FBP (fructose-1,6-bisphosphatase), and TKL (transketolase) in the cells of analyzed O. polymorpha strains from third day of xylose alcoholic fermentation at 45 °C

Strain

Activity U/mg of protein

XR

XDH

XK

PDC

ADH

TKL

FBP

WT

0.012 ± 0.001

0.011 ± 0.001

0.165 ± 0.008

0.103 ± 0.005

0.005 ± 0.002

0.012 ± 0.001

cat8Δ

0.014 ± 0.002

0.006 ± 0.001

0.183 ± 0.012

0.119 ± 0.001

0.008 ± 0.001

0.014 ± 0.003

BEP

0.023 ± 0.003

0.335 ± 0.004

0.494 ± 0.031

0.323 ± 0.018

0.119 ± 0.020

0.012 ± 0.004

0.011 ± 0.001

BEP cat8Δ

0.028 ± 0.002

0.255 ± 0.018

0.629 ± 0.038

0.346 ± 0.006

0.189 ± 0.015

0.019 ± 0.003

0.015 ± 0.002

– Not determined

Table 3

The relative expression levels of the particular genes in the parental strains and cat8Δ mutants at the third day of xylose alcoholic fermentation at 45 °C

ΔΔCt

Genes

XYL1

XYL2

XYL3

PDC1

TKL1

DAS1

TAL1

TAL2

RPE1

FBP1

PCK1

cat8Δ/WT

1.13 ± 0.300

1.05 ± 0.577

2.82 ± 0.438

0.64 ± 0.400

1.10 ± 0.361

2.39 ± 0.342

1.23 ± 0.360

1.21 ± 0.193

2.60 ± 0.486

0.67 ± 0.165

1.10 ± 0.435

BEP cat8Δ/BEP

0.36 ± 0.300

0.62 ± 0.085

1.07 ± 0.086

0.88 ± 0.479

0.79 ± 0.175

0.57 ± 0.195

1.11 ± 0.091

1.12 ± 0.067

1.54 ± 0.052

0.74 ± 0.392

0.76 ± 0.140

BEP/WT

7.66 ± 0.971

18.03 ± 0.045

2.76 ± 0.158

1.96 ± 0.380

1.71 ± 0.178

1.70 ± 0.670

9.29 ± 0.138

3.59 ± 0.138

47.60 ± 0.301

1.02 ± 0.274

0.19 ± 0.414

The mRNA quantification was normalized to ACT1 mRNA

Genes encode: XYL1, xylose reductase; XYL2, xylitol dehydrogenase; XYL3, xylulokinase; PDC1, pyruvate decarboxylase; TKL1, transketolase; DAS1, dihydroxyacetone phosphate synthase or peroxisomal transketolase; TAL1, transaldolase; TAL2, peroxisomal transaldolase; RPE1, ribulosephosphate epimerase; FBP1, fructose-1,6-bisphosphatase; PCK1, phosphoenolpyruvate carboxykinase

Ethanol production by mutants with deletion and overexpression of CAT8 gene in xylose and glucose media

Xylose and glucose fermentation of the isolated cat8Δ and BEP cat8Δ strains was studied under semi-anaerobic conditions (see “Methods” section). It was found that defects of CAT8 gene leads to 1.5-fold increase in ethanol accumulation on the background of the wild-type strain though concentration of the accumulated ethanol was quite low (Table 4; Fig. 2). At the same time, overexpression of CAT8 led to decrease in ethanol production from xylose (Fig. 3). Effect of CAT8 overexpression on glucose fermentation was insignificant (Additional file 4).
Table 4

Main parameters of xylose fermentation at 45 °C by the O. polymorpha strains tested

Strain

Ethanol (g/L)

Ethanol yield (g/g consumed xylose)

Rate of ethanol synthesis (g/g biomass/h)

Productivity of ethanol synthesis (g/L/h)

WTa

0.523 ± 0.054

0.029 ± 0.010

0.009 ± 0.001

0.022 ± 0.001

cat8Δb

0.780 ± 0.083

0.034 ± 0.002

0.012 ± 0.001

0.026 ± 0.001

BEPc

9.620 ± 0.102

0.300 ± 0.011

0.082 ± 0.002

0.169 ± 0.007

BEP cat8Δc

12.51 ± 0.134

0.340 ± 0.015

0.091 ± 0.003

0.205 ± 0.009

a Data of ethanol yield and ethanol (g/L) are represented on YNB medium supplemented with 9% of xylose on the first day (24 h) of fermentation

b 48 h of fermentation

c 72 h of fermentation

Fig. 2

The ethanol production, xylose consumption and biomass accumulation during xylose fermentation at 45 °C of O. polymorpha strains: a WT, b cat8∆, c BEP, d BEP cat8

Fig. 3

The ethanol production of O. polymorpha strains: WT, cat8∆ and strain with overexpression of CAT8 gene (CAT8*) during xylose alcoholic fermentation at 45 °C

It is important to note that deletion of CAT8 in BEP strain also had a positive effect on ethanol accumulation, which increased by 30% and reached 12.5 g ethanol/L. Increased ethanol production from xylose was accompanied by activated xylose consumption from the medium (Fig. 2). Data of Table 4 show that the strain BEP cat8Δ possessed increase in ethanol yield and productivity in xylose medium relative to the parental overproducing strain BEP for 13 and 21%, respectively. Strain BEP cat8Δ did not accumulate xylitol (data not shown) similar to that of the parental strain BEP [16]. Thus, we conclude that Cat8 transcription factor is involved in the control of xylose alcoholic fermentation and the deficiency of this protein activates ethanol production from xylose. In contrast, CAT8 deletion did not have pronounced effect on ethanol production during glucose fermentation both in the wild-type and the BEP strains (Additional file 4). Deletion of CAT8 gene on both wild-type and BEP backgrounds also did not have effects on alcoholic fermentation of sucrose (data not shown).

Discussion

The natural xylose-utilizing thermotolerant yeast O. polymorpha ferments xylose and glucose at highest temperatures known for yeasts, i.e. at 50 °C [6, 8]. The current work introduces CAT8 as a gene involved in the regulation of xylose metabolism and alcoholic fermentation in this organism. Prior to this study, the role of CAT8 in xylose alcoholic fermentation had not been addressed. It was shown that the deletion of this gene in S. cerevisiae slightly activated glucose alcoholic fermentation [30]. In contrast, strong activation was observed in P. guilliermondii [22] though maximally achieved level of ethanol in the latter species was still very low. In O. polymorpha CAT8 deletion did not lead to any significant changes in ethanol production from glucose, while a considerable increase in xylose alcoholic fermentation was observed. The reasons for this difference remain to be elucidated; quite possibly the enzymes involved in ethanol production are not activated in cat8Δ mutants during glucose fermentation. It has also to be pointed out that cell respiration of cat8Δ mutants on xylose was impaired in much higher extent relative to that on glucose as a substrate where BEP cat8Δ showed some increase in glucose respiration (Table 1), assuming xylose redirection from the Krebs cycle and oxidative phosphorylation towards ethanol production. The reason of the increase of ethanol production from xylose by cat8Δ strains could be explained by activation of xylulokinase, alcohol dehydrogenase and ribulosephosphate epimerase (Tables 2, 3) which could be the limiting factors during xylose alcoholic fermentation.

We observed impaired ethanol and glycerol utilization in cat8Δ mutants, suggesting the involvement of CAT8 in regulation of gluconeogenesis in O. polymorpha, similar to that in S. cerevisiae. Remarkably, growth on xylose of cat8Δ mutant isolated from the wild-type strain was also partially impaired which suggests that xylose can be considered, at least partially, as gluconeogenic substrate. i.e., if hexoses are to some extent synthesized from xylose in gluconeogenesis (from glyceraldehyde-3-phosphate which is synthesized in pentose phosphate pathway), this, together with defects in respiration, especially strong on xylose, could cause the redirection of xylose flux of cat8Δ mutants to catabolism and thus the redirection of xylose metabolism to the fermentation mode. Enhanced ethanol production from xylose by cat8Δ mutants could also be explained by the observed increase in enzyme activities and transcriptions of genes involved in xylose utilization and alcoholic fermentation (Tables 2, 3). Contrary, the slight increase in specific activity of fructose-1,6-bisphosphatase in cat8Δ mutants was observed suggesting differences in Cat8 action between S. cerevisiae and O. polymorpha. We suggest that growth impairments of O. polymorpha cat8Δ mutants on glycerol and ethanol are determined by partial defects in respiration which is critical for growth on gluconeogenic substrates. Quite possible that this is also the reason of xylose growth retardation of cat8Δ mutant isolated from the wild-type strain. In spite activity of xylitol dehydrogenase is lowered in cat8Δ mutants, it is unlikely that Xyl2 is the limiting enzyme during growth on xylose as our earlier studies showed that deletion of the main paralog XYL2 (assayed in current manuscript) did not impair growth on xylose at all and deletion of two paralogs of XYL2 impaired growth still not completely [13].

It is interesting to note that overexpression of CAT8 has opposite effect on xylose alcoholic fermentation as compared to that in cat8Δ mutants as transformants overexpressing CAT8 gene were characterized by decrease in ethanol production from xylose (Fig. 3). Apparently high amounts of Cat8 activate xylose gluconeogenesis and respiration while inhibit fermentation of this pentose. Deletion or overexpression of CAT8 had no effect on glucose fermentation suggesting specific involvement of Cat8 protein in regulation of xylose alcoholic fermentation.

Thus, the CAT8 gene is one of the first identified genes specifically involved in regulation of xylose alcoholic fermentation in the natural xylose-fermenting yeasts. Inactivation of this gene (its knock out) increased ethanol production on backgrounds of the wild-type strain and of the advanced ethanol producer from xylose (BEP). The best ethanol producer from xylose described here, accumulated 30% more ethanol relative to the BEP strain from xylose reported previously and 20–25 times more compared to the wild-type strain [16]. The yield and productivity of ethanol synthesis in BEP cat8Δ strain, constructed in this work, for 13 and 21% exceeds those in the reported O. polymorpha ethanol overproducer from xylose. Ethanol yield in the BEP cat8Δ strain (0.34 g/g xylose) is close to that described for S. stipitis (0.35–0.44 g/g xylose) [31] and S. passalidarum (0.42 g/g xylose) [32], however, it was achieved for O. polymorpha at 45 °C whereas the compared organisms are mesophilic and thus cannot grow and ferment at so high temperature. Among thermotolerant ethanol producing strains the promising one is engineered K. marxianus strain with ethanol yield 0.38 g/g xylose at 42 °C, but lower yield at 45 °C (0.27 g/g xylose) [33]. In contrast to recombinant K. marxianus strain [33], BEP cat8Δ did not accumulate byproduct xylitol at all. Still, the level of increase in ethanol synthesis achieved in this work is not enough for feasible ethanol production from xylose. However, we suggest that the described approach could be useful, in combination with other ones, for future construction of the efficient thermotolerant ethanol producers from xylose.

One may assume that cat8Δ mutants of xylose-utilizing recombinant S. cerevisiae could be also characterized by an increase in ethanol production from this pentose. It would also be interesting to check the effects of CAT8 deletion on xylose alcoholic fermentation in the species of natural xylose fermenting yeasts, such as S. stipitis, S. passalidarum and others. We hypothesize that the deletion of CAT8 gene could become a standard approach for development of effective xylose fermenting strains. It would also be of interest to check the role of transcription factors Adr1 [30], and Znf1 [34], Rds2, Sip4 and others [20], in xylose alcoholic fermentation in O. polymorpha and other yeast species. Recently, we checked the effects of the knock-out of two O. polymorpha homologs of transcriptional regulator HAP4, HAP4-A and HAP4-B, on xylose growth and fermentation and found only a slight increase in ethanol production from xylose in hap4-AΔ mutant [35].

We envisage that there are new efficient strategies for additional increase in ethanol production from xylose in O. polymorpha. They include autophagy initiation gene ATG13 [17; Dmytruk, Sibirny, in preparation] and several genes coding for peroxisomal proteins [17; Kurylenko, Ruchala, Vasylyshyn, Dmytruk, Sibirny, in preparation]. Change of expression of the mentioned genes leads to significant and specific increase in ethanol yield from xylose on the background of the wild-type strain. We hope that the manipulation with these gene expression could also be useful for further increase of ethanol production in the described here ethanol overproducer from xylose. Currently our attention is focused to the fermentation of lignocellulosic hydrolysates by constructed xylose fermenting strains. This could constitute an important step towards the establishment of O. polymorpha as a promising high-temperature ethanol producer from xylose and other lignocellulosic sugars.

Conclusions

The mutants of the methylotrophic yeast Ogataea (Hansenula) polymorpha with knock out and overexpression of the ortholog of CAT8 gene coding for transcriptional activator, have been constructed. The cat8Δ mutants showed 30–50% increase in ethanol synthesis from xylose. No effect of CAT8 knock out on ethanol production from glucose was observed. The best strain accumulated 12.5 g of ethanol/L from xylose at 45 °C. Inversely, overexpression of CAT8 resulted in decrease of ethanol production from this pentose.

Methods

Strains, vectors, cultivation condition

The following strains of O. polymorpha were used: NCYC495 leu1-1 (wild-type strain), 2EtOH/XYL1m/XYL2/XYL3/BrPA (designated as BEP from best ethanol producer) which is advanced ethanol producer from xylose isolated by combination of the methods of metabolic engineering and classical selection [16]. Yeast cells were grown on YPD (10 g/L yeast extract, 10 g/L peptone, 20 g/L glucose) or mineral medium (6.7 g/L YNB without amino acids, 20 g/L of carbon source—glucose, xylose, glycerol, ethanol) at 37 °C. For the NCYC495 leu1-1 strain, leucine (40 mg/L) was added to the medium. For the selection of yeast transformants on YPD 0.1 g/L of nourseothricin or 0.35 g/L of hygromycin were added. Alcoholic fermentation of yeast strains was fulfilled by cultivation in liquid mineral medium at oxygen-limited conditions at 37 and 45 °C. The conditions were provided by agitation at 140 rpm. 9% xylose or 9% glucose was added into the medium used for the fermentation. The cells were pregrown in 100 mL of liquid YPX medium (1% yeast extract, 2% peptone and 4% xylose) in 300 mL Erlenmeyer flasks at 220 rpm till the mid-exponential growth phase. Than the cells were precipitated by centrifugation, washed by water and inoculated into 40 mL of the fermentation medium in 100 mL Erlenmeyer flasks covered with cotton plugs. The initial biomass concentration for fermentation experiments was 2 g (dry weight)/L. Fermentations were repeated at least in three independent experiments, each performed in triplicate to ensure the results are reproducible. The bars in the figures indicate the ranges of the standard deviation.

The E. coli DH5α strain (Φ80dlacZΔM15, recA1, endA1, gyrA96, thi-1, hsdR17(r K , m K + ), supE44, relA1, deoR, Δ(lacZYA-argF)U169) was used as a host for plasmid propagation. Strain DH5α was grown at 37 °C in LB medium as described previously [36]. Transformed E. coli cells were maintained on a medium containing 100 mg/L of ampicillin.

Molecular-biology techniques

Standard cloning techniques were carried out as described [36]. Genomic DNA of O. polymorpha was isolated using the Wizard® Genomic DNA Purification Kit (Promega, Madison, WI, USA). Restriction endonucleases and DNA ligase (Fermentas, Vilnius, Lithuania) were used according to the manufacturer specifications. Plasmid isolation from E. coli was performed with the Wizard® Plus SV Minipreps DNA Purification System (Promega, Madison, WI, USA). DNA fragments were separated on a 0.8% agarose (Fisher Scientific, Fair Lawn, NJ, USA) gel. Isolation of fragments from the gel was carried out with a DNA Gel Extraction Kit (Millipore, Bedford, MA, USA). PCR-amplification of the fragments of interest was done with Platinum® Taq DNA Polymerase High Fidelity (Invitrogen, Carlsbad, CA, USA) according to the manufacturer specification. PCRs were performed in GeneAmp® PCR System 9700 thermocycler (Applied Biosystems, Foster City, CA, USA). Transformation of the yeast O. polymorpha was carried out as described previously [37].

Construction and analysis of cat8Δ O. polymorpha deletion mutants

Genomic DNA of O. polymorpha NCYC495 leu 1-1 strain was used as template for isolation of 5′ and 3′ uncoding regions of CAT8 gene by PCR amplifications using primers 5′CAT8 FW/5′CAT8 RW and 3′CAT8 FW/3′CAT8 RW (Sequences of all primers represented in Additional file 5). The resulted 5′CAT8 (671 bp) and 3′CAT8 (697 bp) fragments were EcoRI/BglII or BglII/PstI digested and cloned into EcoRI/PstI linearized vector pUC57. The resulted recombinant was named pUC57-CAT8. Gene natNT2 (1318 bp) conferring resistance to nourseothricin was amplified using vector pRS41N [38] as a template and primers OK19 and OK20. Obtained fragment was BglII-digested and subcloned into BglII-linearized plasmid pUC57-CAT8. As a result of further genetic manipulations recombinant plasmid pUC57-ΔCAT8-natNT2 was constructed (Additional file 1A). After that, plasmid pUC57-ΔCAT8-natNT2 was NdeI-linearized and transformed into O. polymorpha NCYC495 leu1-1 recipient strain using electroporation method. Transformants were selected on the solid YPD medium supplemented with 0.1 g/L of nourseothricin after three days of incubation at 37 °C. Obtained transformants were examined by PCR using genomic DNA of recombinant strains as a template. Transformants with confirmed deletion of CAT8 were stabilized by altering cultivation in nonselective and selective media and once again examined by PCR. Fragments with predicted size were amplified using pairs of primers homologous to the sequence of selective marker and regions outside from the fragments used for recombination (JR_CAT8_FW/OK20 and OK19/JR_CAT8_RW) (Additional file 1C).

Deletion cassette for isolation of cat8Δ mutant on the background of strain BEP was constructed as follows. Genomic DNA of O. polymorpha NCYC495 leu1-1 strain was used as template for isolation of 5′ and 3′ uncoding regions of CAT8 gene by PCR amplifications using primers 5′C8_FW/5′C8_RW and 3′C8_FW/3′C8_RW. The resulted 5′CAT8 (878 bp) and 3′CAT8 (780 bp) fragments were EcoRI/BglII and BglII/PstI double-digested and cloned into EcoRI/PstI linearized vector pUC57. The resulted recombinant was named pUC57-C8. Gene hphNT1 (1777 bp) conferring resistance to hygromycin was amplified from plasmid pRS42H [38] as a template and primers Hyg_FW and Hyg_RW. Obtained fragment was BglII-digested and subcloned into BglII-linearized plasmid pUC57-C8. Resulted plasmid was designated as pUC57-ΔCAT8-hphNT1 (Additional file 1B). Plasmid pUC57-ΔCAT8-hphNT1 was XbaI-linearized and transformed into BEP strain by electroporation. Transformants were selected on the solid YPD medium supplemented with 0.35 g/L of hygromycin after four day of incubation at 37 °C. Homologous recombination of the deletion cassette with target site was verified by PCR applying the same approach as that described above using pairs of primers JR_CAT8_FW/Hyg RW and Hyg FW/JR_CAT8_RW (Additional file 1D).

Construction and analysis of O. polymorpha strains with overexpression of CAT8 gene

Plasmid puc19-GAPp-GAPt-natNT2 [39] was used as the basic one for overexpression of CAT8. Promoter GAP of the gene coding for glyceraldehyde-3-phosphate dehydrogenase was used for CAT8 overexpression. Genomic DNA of O. polymorpha NCYC495 leu1-1 strain was used as template for isolation of CAT8 gene by PCR amplifications using primers C8_F/C8E_R. After that, gene was XbaI/NotI double-degisted and cloned into XbaI/NotI linearized vector puc19-GAPp-NTC. The resulting plasmid was named p19-GAPp-CAT8-GAPt-natNT2 (Additional file 6). Plasmid p19-GAPp-CAT8-GAPt-natNT2 was ScaI-linearized and transformed into NCYC495 leu1-1 strain by electroporation. Transformants were selected on the solid YPD medium supplemented with 0.1 g/L of nourseothricin after three days of incubation at 37 °C. The transformants were stabilized by cultivation in non-selective media with further shifting to the selective media with nourseothricin. The presence of recombinant CAT8 gene driven by the HpGAP promoter in genomic DNA of stable transformants was confirmed by PCR using primers KO644/C8E_R. Overexpression of CAT8 in the resulted strain was confirmed by qRT-PCR (Additional file 3).

Respiration activity assay

Cells were grown to the late exponential phase in mineral medium with glucose or xylose, collected, washed in distilled water and starved in mineral medium without carbon source for 16–18 h. Viability of the starved cells was found to be around 70% of that of the non-starved cells by plate count of colony forming units (data not shown). The respiration rate was measured at 30 °C by Yellow Springs Instrument Co. Clark oxygen electrode (model YSI 5300) in a 5 mL reaction vessel. Determinations were performed in distilled air-saturated water with the concentration of cells 0.5 g/L of dry weight from 5 independent cultivations and started by addition of 1% carbon substrate (glucose, xylose). The respiratory rate was expressed as nanomoles of O2 consumed per minute per mg of cells (dry weight).

Biochemical methods

Samples for enzyme activity measurements were taken from the cultures on the third day of xylose fermentation at 45 °C. The enzyme activity was measured directly after the preparation of cell-free extracts. Protein concentration was determined with Folin reagent [40]. The specific activities of XR, XDH and XK in cell extracts were determined spectrophotometrically as described before [14].

TKL activity was assayed spectrophotometrically at 278 nm as previously described with some modifications [41]. In brief, the reaction mixture contained: 50 mM Tris–HCl buffer (pH 7.5), 2.5 mM MgCl2, 60 μM TPP, cell extract (0.4 mg of protein). The reaction was started by addition of 100 mM glycol aldehyde.

The PDC activity in cell extracts was determined spectrophotometrically according to the method described earlier [15]. The ADH activity was measured by following the reduction of NAD at 340 nm using 96% ethanol as a substrate as described previously [42]. Briefly, the assay mixture contained 100 mM Tris–HCl (pH 8.0), 2 mM NAD, 100 mM ethanol. The reaction was initiated with the addition of cell extract (0.1 mg of protein).

FBP activity was measured spectrophotometrically in cell extracts as described elsewhere with some modifications [43]. Briefly, the FBP assay was performed in a reaction mixture containing 100 mM Tris–HCl buffer (pH 8.5), 1 mM EDTA, 5 mM MgCl2, 2 mM fructose-1,6- diphosphate, 0.4 mM NADP and 1 units of glucose-6-phosphate isomerase and glucose-6-phosphate dehydrogenase. The reaction was initiated with the addition of cell extract (0.4 mg of protein).

All assay experiments were repeated at least twice.

Quantitative real-time PCR (qRT-PCR)

Expression of the XYL1, XYL2, XYL3, DAS1, TAL2, RPE1, TAL1, PDC1, FBP1 and PCK1 genes was analyzed by real-time PCR. Total RNA was extracted using the GeneMATRIX Universal RNA Purification Kit with DNAse I (EURx Ltd., Gdansk, Poland). RNA was quantified using Picodrop Microliter UV/Vis Spectrophotometer and diluted in RNAse free water. The qRT-PCR was performed by 7500 Fast Real-Time PCR System (The Applied Biosystems, USA) with SG OneStep qRT-PCR kit (EURx Ltd., Gdansk, Poland) using gene-specific primer pairs, RNA as a template and ROX reference passive dye according to the manufacturer’s instructions. The primers pairs used for qRT-PCR are listed in Additional file 5: Table S1. Sequences of tested genes were taken from O. polymorpha genome database [28]. In brief, normalized amount of RNA (100 ng) and 0.4 μM of each of the two primers were used in a total reaction volume of 20 μL. The amplification was performed with the following cycling profile: reverse transcription step at 50 °C for 30 min; initial denaturation at 95 °C for 3 min at preparation step; followed by 40 cycles of 15 s at 94 °C and 30 s at 60 °C. Melting curve analysis was performed to verify the specificity and identity of PCR products from 65 to 95 °C in the software of real-time cycler. The amplification for over 35–45 cycles gave abundance of PCR product indicating saturation phase. The fold change of each amplicon in each sample relative to the control sample was normalized to the internal control gene ACT1 and calculated according to the comparative Ct (ΔΔCt) method. All data points were analyzed in triplicate.

Analyses

The biomass was determined turbidimetrically with a Helios Gamma spectrophotometer (OD, 590 nm; cuvette, 10 mm) with gravimetric calibration. Concentrations of xylose and ethanol from fermentation in medium broth were analyzed by HPLC (PerkinElmer, Series 2000, USA) with an Aminex HPX-87H ion-exchange column (Bio-Rad, Hercules, USA). A mobile phase of 4 mM H2SO4 was used at a flow rate 0.6 mL/min and the column temperature was 35 °C. Alternatively, concentrations of ethanol in the medium were determined using alcohol oxidase/peroxidase-based enzymatic kit “Alcotest” [44]. Experiments were performed at least twice.

Abbreviations

BEP: 

best ethanol producer

SSF: 

Simultaneous Saccharification and Fermentation

qRT-PCR: 

quantitative reverse-transcription PCR

XR: 

xylose reductase

XDH: 

xylitol dehydrogenase

XK: 

xylulokinase

TKL: 

transketolase

ADH: 

alcohol dehydrogenase

PDC: 

pyruvate decarboxylase

FBP: 

fructose-1,6-bisphosphatase

Declarations

Authors’ contributions

JR carried out strains construction, evaluation of enzymes activity, respiration activity and qRT-PCR, performed fermentation experiments and co-drafted the manuscript. OOK participated in design of cloning, evaluation of enzymes activity, respiration activity and co-drafted the manuscript. NS commented and approved the manuscript. KVD participated in design of cloning and strains construction, analyzed the date and co-drafted the manuscript. AAS provided guidance and suggestions for experimental design, wrote and edited the manuscript. All authors participated in finalizing the manuscript. All authors read and approved the final manuscript.

Acknowledgements

Not applicable.

Competing interests

The authors declare that they have no competing interests.

Availability of data and materials

The datasets supporting the conclusions of this article are included within the article and its additional files. For other datasets, please contact the corresponding author.

Funding

This work was supported in part by Polish Grant of National Scientific Center (NCN) DEC-2012/05/B/NZ1/01657 awarded to A. Sibirny, FEMS Research Grant FEMS-RG-2015-0096.R1 awarded to J. Ruchala; National Academy of Sciences of Ukraine (Grants 5-17, 6-17 and 35-17) and Science and Technology Center in Ukraine (STCU) (Grant 6188).

Open AccessThis article is distributed under the terms of the Creative Commons Attribution 4.0 International License (http://creativecommons.org/licenses/by/4.0/), which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated.

Authors’ Affiliations

(1)
Department of Biotechnology and Microbiology, University of Rzeszow
(2)
Department of Molecular Genetics and Biotechnology, Institute of Cell Biology
(3)
King Mongkut Technical University

References

  1. Alternative Fuels Data Center. http://www.afdc.energy.gov/data/10331. Accessed 29 Oct 2016.
  2. Hahn-Hägerdal B, Galbe M, Gorwa-Grauslund MF, Lidén G, Zacchi G. Bio-ethanol–the fuel of tomorrow from the residues of today. Trends Biotechnol. 2006;24:549–56.View ArticleGoogle Scholar
  3. Jeffries TW, Jin YS. Metabolic engineering for improved fermentation of pentoses by yeasts. Appl Microbiol Biotechnol. 2004;63:495–509.View ArticleGoogle Scholar
  4. Olofsson K, Bertilsson M, Lidén G. A short review on SSF—an interesting process option for ethanol production from lignocellulosic feedstocks. Biotechnol Biofuels. 2008;1(1):7.View ArticleGoogle Scholar
  5. Nonklang S, Abdel-Banat BMA, Cha-aim K, Moonjai N, Hoshida H, Limtong S, Yamada M, Akada R. High-temperature ethanol fermentation and transformation with linear DNA in the thermotolerant yeast Kluyveromyces marxianus DMKU3–1042. Appl Environ Microb. 2008;74:7514–21.View ArticleGoogle Scholar
  6. Radecka D, Mukherjee V, Mateo RQ, Stojiljkovic M, Foulquié-Moreno MR, Thevelein JM. Looking beyond Saccharomyces: the potential of non-conventional yeast species for desirable traits in bioethanol fermentation. FEMS Yeast Res. 2015;15(6):053.View ArticleGoogle Scholar
  7. Ryabova OB, Chmil OM, Sibirny AA. Xylose and cellobiose fermentation to ethanol by the thermotolerant methylotrophic yeast Hansenula polymorpha. FEMS Yeast Res. 2003;4:157–64.View ArticleGoogle Scholar
  8. Ishchuk OP, Voronovsky AY, Abbas CA, Sibirny AA. Construction of Hansenula polymorpha strains with improved thermotolerance. Biotechnol Bioeng. 2009;104:911–9.View ArticleGoogle Scholar
  9. Peter G, Tornai-Lehoczki J, Shin K-S, Dlauchy D. Ogataea thermophile sp. nov., the teleomorph of Candida thermophila. FEMS Yeast Res. 2007;7:494–6.View ArticleGoogle Scholar
  10. Kata I, Semkiv MV, Ruchala J, Dmytruk KV, Sibirny AA. Overexpression of the genes PDC1 and ADH1 activates glycerol conversion to ethanol in the thermotolerant yeast Ogataea (Hansenula) polymorpha. Yeast. 2016;33(8):471–8.View ArticleGoogle Scholar
  11. Voronovsky AY, Ryabova OB, Verba OV, Ishchuk OP, Dmytruk KV, Sibirny AA. Expression of xylA genes encoding xylose isomerases from Escherichia coli and Streptomyces coelicolor in the methylotrophic yeast Hansenula polymorpha. FEMS Yeast Res. 2005;5:1055–62.View ArticleGoogle Scholar
  12. Voronovsky AY, Rohulya OV, Abbas CA, Sibirny AA. Development of strains of the thermotolerant yeast Hansenula polymorpha capable of alcoholic fermentation of starch and xylan. Metab Eng. 2009;11:234–42.View ArticleGoogle Scholar
  13. Dmytruk OV, Voronovsky AY, Abbas CA, Dmytruk KV, Ishchuk OP, Sibirny AA. Overexpression of bacterial xylose isomerase and yeast host xylulokinase improves xylose alcoholic fermentation in the thermotolerant yeast Hansenula polymorpha. FEMS Yeast Res. 2008;8:165–73.View ArticleGoogle Scholar
  14. Dmytruk OV, Dmytruk KV, Abbas CA, Voronovsky AY, Sibirny AA. Engineering of xylose reductase and overexpression of xylitol dehydrogenase and xylulokinase improves xylose alcoholic fermentation in the thermotolerant yeast Hansenula polymorpha. Microb Cell Fact. 2008;7:21.View ArticleGoogle Scholar
  15. Ishchuk OP, Voronovsky AY, Stasyk OV, Gayda GZ, Gonchar MV, Abbas CA, Sibirny AA. Overexpression of pyruvate decarboxylase in the yeast Hansenula polymorpha results in increased ethanol yield in high-temperature fermentation of xylose. FEMS Yeast Res. 2008;8:1164–74.View ArticleGoogle Scholar
  16. Kurylenko OO, Ruchala J, Hryniv OB, Abbas CA, Dmytruk KV, Sibirny AA. Metabolic engineering and classical selection of the methylotrophic thermotolerant yeast Hansenula polymorpha for improvement of high-temperature xylose alcoholic fermentation. Microb Cell Fact. 2014;13:122.View ArticleGoogle Scholar
  17. Kurylenko O, Semkiv M, Ruchala J, Hryniv O, Kshanovska B, Abbas C, Dmytruk K, Sibirny A. New approaches for improving the production of the 1st and 2nd generation ethanol by yeast. Acta Biochim Pol. 2016;63:31–8.View ArticleGoogle Scholar
  18. Haurie V, Perrot M, Mini T, Jenö P, Sagliocco F, Boucherie H. The transcriptional activator Cat8p provides a major contribution to the reprogramming of carbon metabolism during the diauxic shift in Saccharomyces cerevisiae. J Biol Chem. 2001;276:76–85.View ArticleGoogle Scholar
  19. Hedges D, Proft M, Entian KD. CAT8, a new zinc cluster-encoding gene necessary for derepression of gluconeogenic enzymes in the yeast Saccharomyces cerevisiae. Mol Cell Biol. 1995;15:1915–22.View ArticleGoogle Scholar
  20. Turcotte B, Liang XB, Robert F, Soontorngun N. Transcriptional regulation of nonfermentable carbon utilization in budding yeast. FEMS Yeast Res. 2010;10(1):2–13.View ArticleGoogle Scholar
  21. Watanabe T, Srichuwong S, Arakane M, Tamiya S, Yoshinaga M, Watanabe I, Yamamoto M, Ando A, Tokuyasu K, Nakamura T. election of stress-tolerant yeasts for Simultaneous Saccharification and Fermentation (SSF) of very high gravity (VHG) potato mash to ethanol. Bioresour Technol. 2010;101(24):9710–4.View ArticleGoogle Scholar
  22. Qi K, Zhong JJ, Xia XX. Triggering respirofermentative metabolism in the Crabtree-negative yeast Pichia guilliermondii by disrupting the CAT8 gene. Appl Environ Microbiol. 2014;80:3879–87.View ArticleGoogle Scholar
  23. Randez-Gil F, Bojunga N, Proft M, Entian KD. Glucose derepression of gluconeogenic enzymes in Saccharomyces cerevisiae correlates with phosphorylation of the gene activator Cat8p. Mol Cell Biol. 1997;17:2502–10.View ArticleGoogle Scholar
  24. Georis I, Krijger JJ, Breunig KD, Vandenhaute J. Differences in regulation of yeast gluconeogenesis revealed by Cat8p-independent activation of PCK1 and FBP1 genes in Kluyveromyces lactis. Mol Gen Genet. 2000;264:193–203.View ArticleGoogle Scholar
  25. Ramírez MA, Lorenz MC. The transcription factor homolog CTF1 regulates β-oxidation in Candida albicans. Eukaryot Cell. 2009;8:1604–14.View ArticleGoogle Scholar
  26. Kim OC, Suwannarangsee S, Oh DB, Kim S, Seo JW, Kim CH, Kang HA, Kim JY, Kwon O. Transcriptome analysis of xylose metabolism in the thermotolerant methylotrophic yeast Hansenula polymorpha. Bioprocess Biosyst Eng. 2013;36:1509–18.View ArticleGoogle Scholar
  27. Salusjärvi L, Kankainen M, Soliymani R, Pitkänen JP, Penttilä M, Ruohonen L. Regulation of xylose metabolism in recombinant Saccharomyces cerevisiae. Microb Cell Fact. 2008;7:18.View ArticleGoogle Scholar
  28. Hansenula polymorpha NCYC 495 leu1.1 v2.0—JGI Genome Portal. http://genome.jgi-psf.org/Hanpo2/Hanpo2.home.html. Accessed 27 Oct 2016.
  29. Saraya R, Krikken AM, Kiel JA, Baerends RJ, Veenhuis M, van der Klei IJ. Novel genetic tools for Hansenula polymorpha. FEMS Yeast Res. 2012;12:271–8.View ArticleGoogle Scholar
  30. Watanabe D, Hashimoto N, Mizuno M, Zhou Y, Akao T, Shimoi H. Accelerated alcoholic fermentation caused by defective gene expression related to glucose derepression in Saccharomyces cerevisiae. Biosci Biotechnol Biochem. 2013;77:2255–62.View ArticleGoogle Scholar
  31. Jeffries TW, Grigoriev IV, Grimwood J, Laplaza JM, Aerts A, Salamov A, Schmutz J, Lindquist E, Dehal P, Shapiro H, Jin YS, Passoth V, Richardson PM. Genome sequence of the lignocellulose-bioconverting and xylose-fermenting yeast Pichia stipitis. Nat Biotechnol. 2007;25(3):319–26.View ArticleGoogle Scholar
  32. Long TM, Su YK, Headman J, Higbee A, Willis LB, Jeffries TW. Cofermentation of glucose, xylose and cellobiose by the beetle-associated yeast Spathaspora passalidarum. Appl Environ Microbiol. 2012;78(16):5492–500.View ArticleGoogle Scholar
  33. Zhang J, Zhang B, Wang D, Gao X, Sun L, Hong J. Rapid ethanol production at elevated temperatures by engineered thermotolerant Kluyveromyces marxianus via the NADP(H)-preferring xylose reductase-xylitol dehydrogenase pathway. Metab Eng. 2015;31:140–52.View ArticleGoogle Scholar
  34. Tangsombatvichit P, Semkiv MV, Sibirny AA, Jensen LT, Ratanakhanokchai K, Soontorngun N. Zinc cluster protein Znf1, a novel transcription factor of non-fermentative metabolism in Saccharomyces cerevisiae. FEMS Yeast Res. 2015;15(2):fou002.View ArticleGoogle Scholar
  35. Petryk N, Zhou YF, Sybirna K, Mucchielli MH, Guiard B, Bao WG, Stasyk OV, Stasyk OG, Krasovska OS, Budin K, Reymond N, Imbeaud S, Coudouel S, Delacroix H, Sibirny A, Bolotin-Fukuhara M. Functional study of the Hap4-like genes suggests that the key regulators of carbon metabolism HAP4 and oxidative stress response YAP1 in yeast diverged from a common ancestor. PLoS ONE. 2014;9(12):e112263.View ArticleGoogle Scholar
  36. Sambrook J, Fritsh EF, Maniatis T. Molecular cloning: a laboratory manual. Cold Spring Harbor: Cold Spring Harbor Press; 1989.Google Scholar
  37. Faber KN, Haima P, Harder W, Veenhuis M, Ab G. Highly-efficient electrotransformation of the yeast Hansenula polymorpha. Curr Genet. 1994;25:305–10.View ArticleGoogle Scholar
  38. Taxis C, Knop M. System of centromeric, episomal, and integrative vectors based on drug resistance markers for Saccharomyces cerevisiae. Biotechnique. 2006;40:73–8.View ArticleGoogle Scholar
  39. Yurkiv M, Kurylenko O, Vasylyshyn R, Dmytruk K, Sibirny A. Construction of the efficient glutathione producers in the yeast Hansenula polymorpha, p 323–332. In: Sibirny A, Fedorovyvh D, Gonchar M, Grabek-Lejko D, editors. Living organisms and bioanalytical approaches for detoxification and monitoring of toxic compounds. Rzeszow: University of Rzeszow; 2015. p. 323–33.Google Scholar
  40. Lowry OH, Rosebrough NJ, Farr AL, Randall RJ. Protein measurement with the Folin phenol reagent. J Biol Chem. 1951;193:265–75.Google Scholar
  41. Sevostyanova IA, Solovjeva ON, Kochetov GA. Two methods for determination of transketolase activity. Biochemistry (Mosc). 2006;71(5):560–2.View ArticleGoogle Scholar
  42. Postma E, Verduyn C, Scheffers WA, Van Dijken JP. Enzymic analysis of the crabtree effect in glucose-limited chemostat cultures of Saccharomyces cerevisiae. Appl Environ Microbiol. 1989;55:468–77.Google Scholar
  43. Gancedo JM, Gancedo C. Fructose-1,6-diphosphatase, phosphofructokinase and glucose-6-phosphate dehydrogenase from fermenting and non-fermenting yeasts. Arch Microbiol. 1971;76(2):132–8.Google Scholar
  44. Gonchar MV, Maidan MM, Sibirny AA. A new oxidase-peroxidase kit “Alcotest” for ethanol assays in alcoholic beverages. Food Technol Biotechnol. 2001;39:37–42.Google Scholar

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