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Appl Environ Microbiol. 2004 November; 70(11): 6816–6825. doi: 10.1128/AEM.70.11.6816-6825.2004. | PMCID: PMC525251 |
Copyright © 2004, American Society for Microbiology Saccharomyces cerevisiae Engineered for Xylose Metabolism Exhibits a Respiratory Response Yong-Su Jin,1† Jose M. Laplaza,2 and Thomas W. Jeffries1,2,3* Department of Food Science,1 Department of Bacteriology, University of Wisconsin—Madison,3 Forest Products Laboratory, U.S. Department of Agriculture Forest Service, Madison, Wisconsin2 Received May 12, 2004; Accepted June 24, 2004. Native strains of Saccharomyces cerevisiae do not assimilate xylose. S. cerevisiae engineered for d-xylose utilization through the heterologous expression of genes for aldose reductase (XYL1), xylitol dehydrogenase (XYL2), and d-xylulokinase (XYL3 or XKS1) produce only limited amounts of ethanol in xylose medium. In recombinant S. cerevisiae expressing XYL1, XYL2, and XYL3, mRNA transcript levels for glycolytic, fermentative, and pentose phosphate enzymes did not change significantly on glucose or xylose under aeration or oxygen limitation. However, expression of genes encoding the tricarboxylic acid cycle, respiration enzymes (HXK1, ADH2, COX13, NDI1, and NDE1), and regulatory proteins (HAP4 and MTH1) increased significantly when cells were cultivated on xylose, and the genes for respiration were even more elevated under oxygen limitation. These results suggest that recombinant S. cerevisiae does not recognize xylose as a fermentable carbon source and that respiratory proteins are induced in response to cytosolic redox imbalance; however, lower sugar uptake and growth rates on xylose might also induce transcripts for respiration. A petite respiration-deficient mutant (ρ°) of the engineered strain produced more ethanol and accumulated less xylitol from xylose. It formed characteristic colonies on glucose, but it did not grow on xylose. These results are consistent with the higher respiratory activity of recombinant S. cerevisiae when growing on xylose and with its inability to grow on xylose under anaerobic conditions. Xylose is one of the most abundant carbohydrates in nature. As a structural analog of glucose, it forms the backbone for glucuronoxylans—the predominant hemicellulose of angiosperms ( 44). Many fungi and bacteria will grow on xylose aerobically, but relatively few will produce ethanol from it. Of 689 recognized yeast species, 154 will both ferment glucose and assimilate xylose ( 35), but only 6 of these produce more than trace amounts of ethanol from xylose ( 53). Bacteria employ xylose isomerase (EC 5.3.1.5) to convert d-xylose to d-xylulose, whereas most yeasts, fungi, plants, and animals use aldose (xylose) reductase (EC 1.1.1.21) and xylitol dehydrogenase (EC 1.1.1.9) with xylitol as an intermediate ( 5). When NADPH is a cofactor in the first step, the reaction is tied to NADPH production. The second step is coupled to reduction of NAD +, which can create a cofactor imbalance when oxygen or respiration is limiting ( 4). Naturally occurring yeasts that metabolize xylose anaerobically have an aldose reductase that also accepts NADH ( 56). Yeasts that ferment d-xylose require oxygen for growth on the sugar ( 11, 39). No known native eukaryote will grow on xylose anaerobically. The discovery that yeasts can ferment d-xylulose ( 7, 59) prompted genetic engineering of xylose fermentation in Saccharomyces cerevisiae. Heterologous expression of xylose isomerase ( 1, 36) has had periodic reports of success ( 54), but most efforts have introduced genes coding for xylose reductase ( XYL1), xylitol dehydrogenase ( XYL2) and d-xylulokinase (EC2.7.1.17) ( XYL3 or XKS1) ( 25, 29, 30, 32, 33, 51). Recombinant S. cerevisiae expressing these three genes for xylose assimilation can grow on xylose as a sole carbon source, but its capacity for ethanol production from xylose depends upon oxygen availability. In this respect, its xylose metabolism is similar to those of native xylose-fermenting yeasts ( 18). Very recently, uncharacterized mutations in engineered S. cerevisiae have been shown to impart the capacity for anaerobic growth on xylose ( 50). Metabolic regulation by glucose has been studied in S. cerevisiae for many years ( 16). The regulatory and physiological properties of xylose metabolism have been extensively studied only in the xylose-fermenting yeast Pichia stipitis ( 8, 43), which has served as the source of genes for engineering xylose metabolism in S. cerevisiae. It is crucial to understand the regulatory mechanisms of xylose metabolism, especially if we are to engineer a functional pathway in this nonnative xylose-fermenting organism. In the present study, we used DNA microarrays to investigate how transcriptional regulation of S. cerevisiae differs for xylose and glucose metabolism, and we confirmed the regulation of critical genes by real-time PCR (RT-PCR). We tested two hypotheses rationalizing the low level of production of ethanol from xylose: either growth on xylose does not induce transcripts for glycolytic and fermentative enzymes, or growth on xylose does not repress respiration. As predicted by transcriptional-profiling studies, xylose-grown cells were predominantly aerobic, and we were able to improve xylose fermentation by blocking respiration. Yeast strains and growth conditions. S. cerevisiae YSX3 ( MATα leu2:: LEU2-XYL1 ura3:: URA3-XYL2 Ty3:: NEO-XYL3) was grown in YP medium as described previously ( 30). The cells were grown under full aeration or oxygen limitation, with glucose or xylose as a carbon source (four conditions). The cells were cultivated with full aeration in 200 ml of YP medium with 20 g of either glucose or xylose/liter in 1,000-ml flasks shaken at 300 rpm and were harvested at an optical density at 600 nm (OD 600) of 1. For simulation of real fermentative conditions, oxygen-limited cells were cultivated with an initial OD 600 of 10 in 50 ml of YP medium with 40 g of either glucose or xylose/liter in 125-ml flasks shaken at 100 rpm and were harvested at an OD 600 of 30. For monitoring transcripts in the respiration-deficient mutant, FPL-YSX3P, cells were first grown on YP medium with glucose and harvested at an OD 600 of 1. The harvested cells were transferred into YP medium with xylose, and then RNA was extracted after 24 h of incubation. Residual sugar concentrations were determined by high-performance liquid chromatography ( 30). The cells were centrifuged at 4°C for 3 min, washed once in sterilized water, frozen in liquid nitrogen, and kept at −80°C until RNA extraction. For RT-PCR, cells were grown overnight in YP medium with either 4% xylose or 4% glucose as the carbon source. A 125-ml flask with 50 ml of culture was inoculated to an initial OD 600 of 0.1 and grown at 200 rpm at 30°C to a final optical density of 1.3 to 2.2. The cells were collected by centrifugation, washed, and fast frozen in liquid nitrogen. Concentrations of glucose, xylose, xylitol, xylulose, and ethanol were analyzed by high-performance liquid chromatography (Gilson, Middleton, Wis.). Cell growth was monitored by OD 600. Genomewide expression analysis. GeneChip arrays (Affymetrix, Santa Clara, Calif.) were used to monitor mRNA transcripts of putative S. cerevisiae open reading frames. Quantitative RT-PCR was used to measure expression of P. stipitis XYL1, XYL2, and XYL3 transcripts. Total RNA from yeast cells was isolated as described by Holstege et al. ( 27). cDNA was synthesized with a T7-(dT) 24 primer (GENSET Corp.). Labeling of RNA transcripts, hybridization, and scanning were performed according to the manufacturer's instructions. The mRNA copy number per cell was calculated using the hybridization signal obtained from the GeneChip software, assuming that there are 15,000 mRNA molecules per yeast cell ( 20). RT-PCR. Cells from four independent cultures were used for each condition. mRNA was extracted following the protocol described by Holstege et al. ( 27). cDNA was constructed using random oligonucleotides and the Reverse Transcription System kit (Promega). RT-PCR analyses of the samples were done with SYBR Green PCR Master Mix (Applied Biosystems) as recommended by the manufacturer, except that 15 pmol of oligonucleotides and a final volume of 25 μl per reaction were used. Genomic DNA of YSX3 was extracted as described by Jin et al. ( 31) and used for a standard curve. Actin was used to normalize for mRNA concentration. All data points were done in triplicate. A Student t test was used to determine if the samples were statistically significant at a 95% confidence level. Data analysis and databases. The DNA-Chip Analyzer (dChip) program ( http://www.dchip.org) was used to analyze data from the GeneChip instrument. One culture condition (glucose under high aeration) was repeated to assess reproducibility and to determine the criteria for comparing mRNA levels under different culture conditions. Of 5,944 genes, the mRNA levels of 120 genes (2%) changed more than twofold between replicates. However, the greatest variations were observed for genes expressed at fewer than two copies per cell. To consider only significant transcript changes, we filtered out genes whose mRNA signals changed less than twofold and that were present at fewer than two copies per cell ([mRNA] Experiment/[mRNA] Base > 2 and |[mRNA] Experiment − [mRNA] Base| > 2 copies). By these criteria, if a transcript was present at more than two copies per cell and if its signal changed at least twofold in intensity, we had a 99.7% assurance that the change was significant. To facilitate easier data mining, we constructed a relational database between the GeneChip data and other on-line databases, such as the Saccharomyces genome database ( http://genome-www.stanford.edu/Saccharomyces/), the Proteome Database ( 26), and the Comprehensive Yeast Genome Database at the Munich Information Center for Protein Sequences ( http://mips.gsf.de/proj/yeast/CYGD/db/index.html). Hierarchical clustering analysis and visualization were performed using the Cluster and TreeView programs developed by Eisen et al. ( 12). Expression data are deposited on the Entrez GEO database ( http://www.ncbi.nlm.nih.gov/geo). The series ordered group is GSE835. We mapped our expression data to a compiled transcriptional regulatory network using the methods of Herrgård et al. ( 22, 23). Induction of respiration deficiency. S. cerevisiae FPL-YSX3 (10 7 cells/ml) was treated with 20 μg of ethidium bromide/ml in YPD ( 30). The flask was wrapped with aluminum foil and incubated at 30°C for 24 h. The cells were cultivated again in YPD with ethidium bromide and then plated in YPD agar. Following isolation, the absence of respiration activity was verified with a Clark-type oxygen electrode, as described by Jin et al. ( 29). Doubling times were ~2.7 and 8 h for cells grown on glucose and 4.7 and 16 h for cells grown on xylose under aerobic and oxygen-limited conditions, respectively. For all four conditions, residual sugar was present at the time of harvest. No ethanol was detected under the high-aeration conditions, whereas ethanol was detected under oxygen-limited conditions. Although some small amount of ethanol might have been formed under the high-aeration conditions on glucose, the cells were not carbon limited under the low-aeration, high-carbon, and high-cell-density conditions. Transcriptional reprogramming with response to carbon source and aeration change. Oxygen availability did not significantly control gene expression in cells grown on glucose, whereas it greatly affected expression in cells grown on xylose. Of the 5,944 genes detected under the four different culture conditions, only 290 (5%) were differentially expressed under aerobic and oxygen-limited conditions on glucose. In contrast, 509 genes (8.7%) showed differential expression under aerobic and oxygen-limited conditions on xylose (Table 1). The 785 genes whose mRNA levels changed significantly between any two out of the four culture conditions were classified into their functional categories. Genes involved in energy production changed the most (Fig. ). More than 40% of all genes involved in energy production changed more than twofold in the glucose oxygen-limited (GOL) versus xylose oxygen-limited (XOL) comparison. Genes involved in amino acid metabolism, translation, stress, and defense also changed significantly. Patterns of expression levels identified genes with similar responses over the four different cultivation conditions ( 6). Although respiration-related genes were coregulated, cluster analysis did not clearly discriminate genes that function together physiologically. Transcript levels for MTH1, encoding a repressor of hexose transport genes ( 47), and HAP4, encoding the CCAAT binding protein ( 3), increased significantly on xylose under aerobic or oxygen-limited conditions. Overexpression of Hap4p causes cells to enter a hyperrespiratory state ( 37). | TABLE 1.Numbers of genes showing >2-fold differences under different conditions |
mRNA levels of XYL1 and XYL2 changed significantly in response to culture conditions (Fig. ). While these two genes were under the control of the same promoter ( TDH1), they exhibited different patterns of expression over the four culture conditions. The mRNA level of XYL3 was much lower than those of XYL1 and XYL2. Transcription of XYL3 was driven by its native P. stipitis promoter, which does not have cis-acting regulatory sequences native to S. cerevisiae and is considerably weaker than the TDH1 promoter in S. cerevisiae ( 30). Engineered S. cerevisiae increases transport, TCA, and gluconeogenic transcripts on xylose. Transcript levels of most genes did not change significantly with respect to carbon sources (Fig. ), even though glucose was metabolized much faster than xylose. Expression of HXK1 increased >7-fold when cells were grown on xylose, regardless of aeration conditions. Hexokinase PI (Hxk1p) is induced when cells are grown on nonfermentable carbon sources ( 21), which suggests that recombinant S. cerevisiae recognizes xylose as a nonfermentable carbon source. Clearly, the mRNA levels of genes encoding the tricarboxylic acid (TCA) cycle and respiration pathway enzymes increased during xylose metabolism, and they were induced to a greater extent under oxygen-limited rather than fully aerobic conditions. These genes were repressed regardless of the aeration conditions during glucose metabolism. The expression of the one exception, CIT2, which codes for citrate synthase, was relatively higher on glucose. Genes for the pentose phosphate pathway were mostly unchanged, except for TKL2, which was induced many-fold on xylose from a low level, and GND2, which was induced on xylose under oxygen-limited conditions. Transcripts for the gluconeogenic enzymes, encoded by GDH2, ICL1, PCK1, and FBP1, were induced 3.4-, 4-, 3.3-, and 7-fold, respectively, when grown aerobically on xylose compared to growth on glucose. Interestingly, PCK1 was induced to an even greater extent by xylose under oxygen-limiting conditions. Transcripts for several enzymes in the lower half of the glycolytic pathway, most notably those encoded by GPM2, ENO2, and PYK1 ( CDC19), were significantly higher in cells grown on glucose than in those grown on xylose. Even though the fermentative enzymes for ethanol production did not change significantly on the two carbon sources, transcripts of enzymes for ethanol oxidation (encoded by ADH2, ALD3, and ACS1) all increased significantly on xylose (Fig. ). Xylose transport may limit xylose fermentation in recombinant S. cerevisiae YSX3, because it does not have high-affinity transporters for xylose, as is thought to be the case for native xylose-fermenting yeast. Hexose transporters in S. cerevisiae transport xylose, but with less specificity and at a lower rate than with glucose ( 19). Of the 17 known hexose transporters, those encoded by HXT1, HXT2, HXT3, HXT4, HXT5, HXT6, and HXT7 were differentially expressed under all four conditions (Table 2). Transcription of the low-affinity HXT1 and HXT3 transporters is induced by high glucose concentrations ( 45). We confirmed that mRNA levels of HXT1 and HXT3 were higher in the cell during growth on glucose. Induced transcription of HXT2 during growth on xylose at high aeration was unexpected, because HXT2 and HXT4 are expressed at low levels in cells growing either in the absence of glucose or on high glucose concentrations ( 45). Transcription of the high-affinity HXT6 and HXT7 transporters were strongly derepressed on xylose, as they are on other nonfermentable carbon sources ( 34). | TABLE 2.mRNA levels of hexose transporters under different culture conditions |
Expression of genes for mitochondrial redox shuttle and Hap4p. Yeast cells can maintain a neutral redox balance in the cytosol during glucose fermentation by coupling NAD + reduction in the glyceraldehyde-3-phosphate dehydrogenase (GAPDH) reaction to the alcohol dehydrogenase (ADH) reaction, but cells confront a redox imbalance during xylose fermentation because of a cofactor difference between the xylose reductase and xylitol dehydrogenase reactions. The transcript levels of genes for known NAD +/NADH shuttle systems—particularly NDI1, NDE1, GPD1, and GUT1—increased significantly during xylose metabolism and were even higher under oxygen-limited conditions than under aerobic conditions. This suggests that NAD +/NADH shuttle systems are responsive to the cytosolic and mitochondrial redox balances during xylose metabolism (Fig. ). The transcriptional activator Hap2/3/4/5 complex induces expression of respiratory genes. When S. cerevisiae is grown on nonfermentable carbon sources, the complex binds to the CCAAT box, which is usually found upstream of respiratory genes ( SPR3, COX6, QCR8, and CYC1) ( 41). We profiled the mRNA levels of each transcriptional factor in the Hap2/3/4/5 complex under all four culture conditions (Fig. ). Of the four transcriptional factors, mRNA of HAP4 increased most significantly during xylose metabolism, which is consistent with previous findings that Hap4p is the main regulator of this complex ( 15). HAP4 transcript levels were severalfold higher on xylose than on glucose and were highest under oxygen-limited conditions. When we compared the expression analysis data that we obtained in GeneChip studies to those from separate experiments performed with RT-PCR, the two methods led to nearly identical results (Table 3). Where GeneChip studies showed significant differences in transcript levels of cells grown on glucose and on xylose, these same significant differences were detected by RT-PCR. In most instances, however, the magnitudes of the changes appeared to be greater in the RT-PCR experiments. In one case ( NDE1), the Affymetrix data did not show a significant difference between the xylose-grown and glucose-grown transcript levels, and the RT-PCR results did show a difference. However, the Affymetrix and RT-PCR changes were each in the same direction (increased expression on xylose), and the significant change indicated by RT-PCR reinforced our overall hypothesis that growth on xylose induces higher levels of respiration-related transcripts. | TABLE 3.Comparison of expression analysis data from Affymetrix and RT-PCR determinations of selected transcripts |
Redirecting metabolic flux to ethanol by respiration deficiency. Transcript levels clearly indicated that xylose metabolism in recombinant S. cerevisiae was oxidative, because TCA cycle and respiration genes were not repressed by xylose. As a result, metabolic flux at the pyruvate branch point favored respiration over ethanol production. Therefore, we increased the metabolic flux into ethanol production by blocking respiration in S. cerevisiae. Because S. cerevisiae is a petite-positive yeast, a cytoplasmic petite mutant could be isolated by treatment with ethidium bromide. The parental strain (FPL-YSX3) consumed oxygen at a rate of 29.61 ± 1.65 μmol (g of cells  · min) −1, while the petite mutant (FPL-YSX3P) did not consume a measurable amount of oxygen (data not shown). We also tested the growth of the petite mutant on glucose and xylose. Interestingly, the YSX3P mutant grew on glucose, but it could not grow on xylose. This result was consistent with previous observations that S. cerevisiae cannot grow anaerobically on xylulose ( 38) and that xylose-fermenting yeast cannot grow on xylose under anaerobic conditions ( 49). Transcript analysis of FPL-YSX3P showed that all of the respiration-related genes that were elevated two- to threefold in FPL-YSX3 grown on xylose were down-regulated in the petite mutant. Levels of GND2, HXT5, ADH2, and HXK1 transcripts were higher in FPL-YSX3P than in FPL-YSX3 when both strains were grown on glucose. ADH2 and HXK1 are normally repressed by glucose. When grown on xylose, FPL-YSX3P showed higher levels of HXT5, HXT16, HXT1, and HXT4 than FPL-YSX3. Although the respiration-deficient mutant (FPL-YSX3P) could not grow on xylose, it showed improved fermentation capacity relative to its parental strain and produced more ethanol from a mixture of glucose and xylose (Table 4). The maximum ethanol concentration was 1.3-fold greater with FPL-YSX3P than with FPL-YSX3 (Fig. ). Petite cells that were pregrown on glucose showed specific ethanol production rates on xylose more than three times higher than those of the parental strain (0.043 versus 0.013 g of ethanol g of cells −1 h −1). The mutant produced more ethanol and accumulated less xylitol from xylose. The maximum ethanol concentrations produced from 40 g of xylose/liter were 5.4 and 10.7 g of ethanol/liter for FPL-YSX3 and FPL-YSX3P, respectively. The ethanol yield increased significantly (from 0.12 to 0.29 g of ethanol/g of xylose), and the xylitol yield decreased slightly (from 0.55 to 0.46 g of xylitol/g of xylose). | TABLE 4.Comparison of sugar consumptions and product yields (xylitol, glycerol, acetate, and ethanol) after 72 ha |
Integrating gene expression data into the known regulatory network in yeast. To investigate whether our expression data are compatible with known regulatory effects in yeast and to summarize the data, we superimposed our expression results onto a network of interactive effectors, regulators, and enzymes. We obtained a physical-interaction network with 311 elements from Herrgård et al. ( 23). This represents a known metabolic network, including small molecule effectors, environmental factors, transcriptional activators, and the genes that they regulate (Fig. ). We found moderately good correlation between our expression data and the interactions described in the network. Respiration-related transcriptional activators and the genes regulated by these transcriptional factors were expressed more when cells were grown on xylose than when they were grown on glucose. Most transcriptional factors and genes related to amino acid synthesis were expressed more when cells were grown on glucose. In contrast, the GCN4 transcript level was slightly higher on xylose than on glucose. This confirms previous findings that regulation of Gcn4p occurs at the level of translation rather than transcription ( 24). Our experiments were designed to test the effects of two carbon sources and two aeration conditions on the expression profile of engineered S. cerevisiae. To accommodate the physiological changes associated with the different capacities of the cells, other experimental variables were also altered. Cell densities were lower under the high-aeration conditions and higher under the low-aeration conditions to achieve oxygen saturation for full respiration and oxygen limitation for fermentation, respectively. Glucose and xylose concentrations were higher under low aeration to accommodate the higher sugar uptake associated with fermentation ( 30). While these changes introduced additional variables, the dominant effect was to lower the specific oxygen uptake rate under the low-aeration, high-cell-density conditions. We harvested cells in mid-growth phase under each of the four conditions. Oxygen transfer limits cell growth at very high cell densities. van Hoek et al. showed that with S. cerevisiae the fermentative capacity of the cells correlates strongly with the growth rate ( 55). One might therefore expect to see lower ethanol production rates because growth rates were lower under the low-aeration, high-cell-density conditions. We observed higher growth rates under the fully aerobic conditions than under the oxygen-limited conditions, yet we observed ethanol only under oxygen limitation. These results are consistent with higher sugar uptake as a consequence of higher aeration. It is possible that the low cell densities used under high aeration simply did not generate detectable levels of ethanol. While the cell densities differed by 30-fold between the aerobic and oxygen-limited conditions, even at the highest cell density (OD 600 of 30 ≈ 7.5 g [dry weight] of cells/liter) the medium was not limiting growth, so the dominant effect observed was the comparison of fully aerobic growth with oxygen-limited respirofermentative growth. S. cerevisiae engineered for xylose metabolism clearly did not exhibit a fermentative response to the sugar even under oxygen-limited conditions. In fact, transcript levels for HAP4 and the respiratory proteins that it regulates increased on xylose even as oxygen availability decreased. Many previous studies have examined global transcript levels after environmental and cellular perturbations of S. cerevisiae. These include the diauxic shift ( 9), galactose induction ( 46), aerobic-anaerobic cultivation ( 52), mutations in transcriptional apparatus ( 27), and loss of mitochondrial function ( 14). Most have used glucose or some carbon sources that are naturally metabolized. Here, we report the expression response of S. cerevisiae harboring a complete nonnative xylose metabolic pathway from P. stipitis. Even though the capacity for xylose assimilation was functional, the regulatory network for xylose fermentation was not adequate. It is not clear whether this was due to the absence of specific signal pathways or to other more general regulatory mechanisms. We conclude that when engineering novel metabolic capacity in a heterologous host, it is not sufficient to provide the enzymes for a particular pathway; the rest of the metabolic system must function in a coordinated manner as well. Two other research groups have recently published papers describing transcriptional profiles in recombinant S. cerevisiae during xylose metabolism. Wahlbom et al. ( 58) used chemostats to cultivate cells for mRNA measurements. They compared the levels of transcripts of S. cerevisiae TMB 3399 and TMB 3400 when grown on glucose, glucose plus xylose, or (for TMB 3400) xylose alone. Sedlak et al. ( 48) examined batchwise fermentation of glucose-xylose mixtures by S. cerevisiae 424A(LNH-ST). The present study performed batch fermentations with S. cerevisiae YSX3 using either glucose or xylose alone. Although the other two data sets are not published on line to enable complete comparisons, all three studies found that genes coding for glycolytic enzymes were not significantly affected by the carbon source and that the mRNA levels of XKS1, coding for endogenous xylulokinase, were higher in cells grown on xylose alone, whereas they were repressed in the presence of glucose either alone or when present along with glucose. Wahlbom et al. ( 58) and the present study showed that genes for gluconeogenesis and the glyoxylate pathway ( PCK1 and ICL1) are highly expressed in cells grown on xylose. Both groups also reported that transcripts for galactose metabolism were derepressed in the TMB 3400 cells growing on xylose alone. There are also some discrepancies. For instance, in the chemostat studies of Wahlbom et al. ( 58), the transcript level of HXK1 was higher in cells grown on glucose than in those grown on xylose, whereas in our present studies using batch fermentation, the transcript level of HXK1 was much higher on xylose than on glucose ( 48). In a glucose-limited chemostat, where the glucose concentration is very low, cells could be in a glucose-derepressed state. Thus, the glucose-limited chemostat culture experiment might not have monitored derepression of HXK1 during the transition of carbon sources from glucose to xylose. In contrast, our cells, which were grown on glucose in batch culture, were under glucose-repressed conditions. Recently Belinchon and Gancedo showed that xylose could cause moderate carbon catabolite repression in S. cerevisiae TMB3001, a strain that has been engineered for xylose metabolism ( 2). In that study, growth on 1% xylose induced NAD-dependent glutamate dehydrogenase ~24-fold over the level attained with 2% glucose. Activities of fructose-1,6 bisphosphatase and isocitrate lyase on 2% xylose were significantly lower than those attained with growth on ethanol but much higher than those seen with growth on glucose. These results were consistent with our findings and those of Wahlbom et al. ( 58) that growth of engineered S. cerevisiae on xylose induces transcripts for gluconeogenesis. S. cerevisiae expresses the high-affinity transporters Hxt6p and Hxt7p when growing on glucose or fructose but not on galactose or ethanol, and the low-affinity transporter Hxt1p is induced only at high dilution rates or during the initial phases of batch fermentation on glucose ( 10). Our studies showed that transcripts of HXT6 and HXT7 were strongly induced on xylose but not on glucose and that HXT1 was induced at a much higher level on glucose than on xylose. Our findings are consistent with a role for xylose as a nonrepressing carbon source that does not trigger induction of low-affinity uptake systems. It is also possible that cells increased production of respiratory transcripts in response to a low level of sugar uptake. By introducing multiple permease genes, Goffrini et al. enabled Kluyveromyces lactis to grow on galactose and raffinose without respiration ( 17). Ostergaard et al. were able to increase galactose consumption and respirofermentative activity in S. cerevisiae by altering the regulatory network of the cell ( 42). If this is the case, overexpression of a xylose transporter might reduce the induction of respiration-related transcripts. We were able to confirm the Crabtree effect at the level of transcription. This regulatory pattern is characterized by a tight repression of TCA cycle enzymes (encoded by ACO1, IDH2, KGD1, SDH1, and MDH1) and respiratory enzymes (encoded by QCR2 and COX5A) by glucose even under aerobic conditions. We also verified the known regulation of gene expression by oxygen. The mRNA levels of Hap4p, a critical component of the transcriptional activator complex Hap2/3/4, increased threefold under aerobic conditions, even with glucose as a carbon source (Fig. ). We also discovered unexpected changes in mRNA levels under those conditions. For instance, the mRNA levels of HXK1, FBP1, and PCK1 increased significantly when cells were grown on xylose, regardless of aeration. Expression of these genes is known to increase when cells are grown on nonfermentable carbon sources (Fig. ). Moreover, the expression of TCA cycle enzymes and respiratory enzymes was not repressed by xylose in the same manner as glucose. Combining these results, we can conclude that recombinant S. cerevisiae does not recognize xylose as a fermentable carbon source. This supports the repression hypothesis—that xylose is poorly metabolized into ethanol because it does not repress respiration in the manner of glucose—rather than the induction hypothesis. In contrast, the induction hypothesis—that xylose does not induce the expression of fermentative enzymes—is not supported, because we observed that mRNA levels of fermentative enzymes (encoded by ADH1 and PDC1) did not change in response to the carbon source. Additional experiments will be necessary to determine whether increased sugar transport can reduce the induction of respiratory transcripts. Another notable result was that the expression of many oxidoreductases using NADH or NADPH as cofactors increased when cells were grown on xylose. mRNA levels of GDH2, encoding glutamate dehydrogenase, and LYS12, encoding homoisocitrate dehydrogenase, increased significantly when cells were grown on xylose. These enzymes might work to alleviate redox imbalance during xylose metabolism. It might be possible to change the intracellular redox balance by overexpressing GDH2; Nissen et al. ( 40) showed that the product formation pattern could be changed (glycerol to ethanol) under anaerobic conditions by oxidizing surplus NADH and overexpression of GDH2 in a gdh1 mutant. Genetic approaches to improving xylose utilization have mostly focused on blocking the oxidative and enhancing the nonoxidative phases of the pentose phosphate pathway ( 28). This reduces xylitol production by decreasing the supply of NADPH, but it also greatly inhibits xylose assimilation. In the approach used here, we blocked the terminal oxidation of NADH by respiration, thereby redirecting reductant into ethanol production. However, the respiration-deficient mutant YSX3P (ρ°) did not grow on xylose despite being able to ferment the sugar at an elevated rate. This observation is consistent with previous reports. Maleszka and Schneider ( 38) found that S. cerevisiae required oxygen for growth on d-xylulose and that petite mutants of S. cerevisiae did not grow on d-xylulose. Likewise, S. cerevisiae metabolically engineered with XYL1, XYL2, and XKS1 did not grow on xylose as a sole carbon source under anaerobic conditions ( 13). Recent studies have shown that mutants of recombinant S. cerevisiae that show some limited growth on xylose under anaerobic conditions can be obtained through continuous culture ( 50). While this evolutionary engineering approach is promising, the natures of these mutants are still unknown. Despite several attempts, we have not been able to obtain significant growth of the petite mutants on xylose with minimal medium. It is possible that the complete loss of the mitochondrial genome, as occurs in ρ° mutants, deletes physiological functions other than respiration that are essential for anaerobic growth on xylose. However, the petite strain could sustain viability on xylose, and the specific xylose uptake rate of the mutant was 50% higher than that of its parent (0.081 versus 0.054 g of xylose g of cells −1 h −1). This is one of the essential characteristics of cells metabolically engineered for industrial fermentations. This research was supported by USDA/NRICGP grant no. 2001-35504-10695 to T.W.J. We express our profound gratitude to Marcus Herrgård for providing the transcriptional regulatory network database. 1. Amore, R., M. Wilhelm, and C. P. Hollenberg. 1989. The fermentation of xylose—an analysis of the expression of BacillusBacillus and ActinoplanesActinoplanes xylose isomerase genes in yeast. Appl. Microbiol. Biotechnol. 30:351-357. 2. Belinchon, M. M., and J. M. Gancedo. 2003. Xylose and some non-sugar carbon sources cause catabolite repression in Saccharomyces cerevisiaeSaccharomyces cerevisiae. Arch. Microbiol. 180:293-297. [PubMed] 3. Brons, J. F., M. De Jong, M. Valens, L. A. Grivell, M. Bolotin-Fukuhara, and J. Blom. 2002. Dissection of the promoter of the HAP4HAP4 gene in S. cerevisiaeS. cerevisiae unveils a complex regulatory framework of transcriptional regulation. Yeast 19:923-932. [PubMed] 4. Bruinenberg, P. M., P. H. M. de Bot, J. P. van Dijken, and W. A. Scheffers. 1983. The role of redox balances in the anaerobic fermentation of xylose by yeasts. Eur. J. Appl. Microbiol. Biotechnol. 18:287-292. 5. Chiang, C., and S. G. Knight. 1960. The metabolism of d-xylose by moulds. Nature 188:79-80. [PubMed] 6. Chiang, D. Y., P. O. Brown, and M. B. Eisen. 2001. Visualizing associations between genome sequences and gene expression data using genome-mean expression profiles. Bioinformatics 17(Suppl. 1):S49-S55. [PubMed] 7. Chiang, L.-C., C.-S. Gong, L.-F. Chen, and G. Taso. 1981. d-Xylulose fermentation by Saccharomyces cerevisiaeSaccharomyces cerevisiae. Appl. Environ. Microbiol. 42:284-289. 8. Cho, J. Y., and T. W. Jeffries. 1999. Transcriptional control of ADHADH genes in the xylose-fermenting yeast Pichia stipitisPichia stipitis. Appl. Environ. Microbiol. 65:2363-2368. [PubMed] 9. DeRisi, J. L., V. R. Iyer, and P. O. Brown. 1997. Exploring the metabolic and genetic control of gene expression on a genomic scale. Science 278:680-686. [PubMed] 10. Diderich, J. A., M. Schepper, P. van Hoek, M. A. Luttik, J. P. van Dijken, J. T. Pronk, P. Klaassen, H. F. Boelens, M. J. de Mattos, K. van Dam, and A. L. Kruckeberg. 1999. Glucose uptake kinetics and transcription of HXTHXT genes in chemostat cultures of Saccharomyces cerevisiaeSaccharomyces cerevisiae. J. Biol. Chem. 274:15350-15359. [PubMed] 11. du Preez, J. C., B. A. Prior, and A. M. T. Monteiro. 1984. The effect of aeration on xylose fermentation by Candida shehataeCandida shehatae and Pachysolen tannophilusPachysolen tannophilus—a comparative study. Appl. Microbiol. Biotechnol. 19:261-266. 12. Eisen, M. B., P. T. Spellman, P. O. Brown, and D. Botstein. 1998. Cluster analysis and display of genome-wide expression patterns. Proc. Natl. Acad. Sci. USA 95:14863-14868. [PubMed] 13. Eliasson, A., C. Christensson, C. F. Wahlbom, and B. Hahn-Hägerdal. 2000. Anaerobic xylose fermentation by recombinant Saccharomyces cerevisiaeSaccharomyces cerevisiae carrying XYL1XYL1, XYL2XYL2, and XKS1XKS1 in mineral medium chemostat cultures. Appl. Environ. Microbiol. 66:3381-3386. [PubMed] 14. Epstein, C. B., J. A. Waddle, W. T. Hale, V. Dave, J. Thornton, T. L. Macatee, H. R. Garner, and R. A. Butow. 2001. Genome-wide responses to mitochondrial dysfunction. Mol. Biol. Cell 12:297-308. [PubMed] 15. Forsburg, S. L., and L. Guarente. 1989. Identification and characterization of Hap4: a third component of the CCAAT-bound Hap2/Hap3 heteromer. Genes Dev. 3:1166-1178. [PubMed] 16. Gancedo, J. M. 1998. Yeast carbon catabolite repression. Microbiol. Mol. Biol. Rev. 62:334-361. [PubMed] 17. Goffrini, P., I. Ferrero, and C. Donnini. 2002. Respiration-dependent utilization of sugars in yeasts: a determinant role for sugar transporters. J. Bacteriol. 184:427-432. [PubMed] 18. Grootjen, D. R. J., R. G. J. M. van der Lans, and K. C. A. M. Luyben. 1990. Effects of the aeration rate on the fermentation of glucose and xylose by Pichia stipitisPichia stipitis CBS-5773. Enzyme Microb. Technol. 12:20-23. 19. Hamacher, T., J. Becker, M. Gardonyi, B. Hahn-Hägerdal, and E. Boles. 2002. Characterization of the xylose-transporting properties of yeast hexose transporters and their influence on xylose utilization. Microbiology 148:2783-2788. [PubMed] 20. Hereford, J. B., and M. Rosbash. 1977. Number and distribution of poly-adenylated RNA sequences in yeast. Cell 10:453-462. [PubMed] 21. Herrero, P., J. Galindez, N. Ruiz, C. Martinez-Campa, and F. Moreno. 1995. Transcriptional regulation of the Saccharomyces cerevisiae HXK1Saccharomyces cerevisiae HXK1, HXK2HXK2 and GLK1GLK1 genes. Yeast 11:137-144. [PubMed] 22. Herrgård, M. J., M. W. Covert, and B. O. Palsson. 2003. Reconciling gene expression data with known genome-scale regulatory network structures. Genome Res. 13:2423-2434. [PubMed] 23. Herrgård, M. J., M. W. Covert, and B. O. Palsson. 2004. Reconstruction of microbial transcriptional regulatory networks. Curr. Opin. Biotechnol. 15:70-77. [PubMed] 24. Hinnebusch, A. G. 1997. Translational regulation of yeast GCN4.GCN4. A window on factors that control initiator-tRNA binding to the ribosome. J. Biol. Chem. 272:21661-21664. [PubMed] 25. Ho, N. W. Y., Z. D. Chen, and A. P. Brainard. 1998. Genetically engineered SacccharomycesSacccharomyces yeast capable of effective cofermentation of glucose and xylose. Appl. Environ. Microbiol. 64:1852-1859. [PubMed] 26. Hodges, P. E., W. E. Payne, and J. I. Garrels. 1998. The Yeast Protein Database (YPD): a curated proteome database for Saccharomyces cerevisiae.Saccharomyces cerevisiae. Nucleic Acids Res. 26:68-72. [PubMed] 27. Holstege, F. C., E. G. Jennings, J. J. Wyrick, T. I. Lee, C. J. Hengartner, M. R. Green, T. R. Golub, E. S. Lander, and R. A. Young. 1998. Dissecting the regulatory circuitry of a eukaryotic genome. Cell 95:717-728. [PubMed] 28. Jeppsson, M., B. Johansson, B. Hahn-Hägerdal, and M. F. Gorwa-Grauslund. 2002. Reduced oxidative pentose phosphate pathway flux in recombinant xylose-utilizing Saccharomyces cerevisiaeSaccharomyces cerevisiae strains improves the ethanol yield from xylose. Appl. Environ. Microbiol. 68:1604-1609. [PubMed] 29. Jin, Y. S., S. Jones, N. Q. Shi, and T. W. Jeffries. 2002. Molecular cloning of XYL3XYL3 (d-xylulokinase) from Pichia stipitisPichia stipitis and characterization of its physiological function. Appl. Environ. Microbiol. 68:1232-1239. [PubMed] 30. Jin, Y. S., T. H. Lee, Y. D. Choi, Y. W. Ryu, and J. H. Seo. 2000. Conversion of xylose to ethanol by recombinant Saccharomyces cerevisiaeSaccharomyces cerevisiae containing genes for xylose reductase and xylitol dehydrogenase from Pichia stipitisPichia stipitis. J. Microbiol. Biotechnol. 10:564-567. 31. Jin, Y. S., H. Ni, J. M. Laplaza, and T. W. Jeffries. 2003. Optimal growth and ethanol production from xylose by recombinant Saccharomyces cerevisiaeSaccharomyces cerevisiae require moderate d-xylulokinase activity. Appl. Environ. Microbiol. 69:495-503. [PubMed] 32. Johansson, B., C. Christensson, T. Hobley, and B. Hahn-Hägerdal. 2001. Xylulokinase overexpression in two strains of Saccharomyces cerevisiaeSaccharomyces cerevisiae also expressing xylose reductase and xylitol dehydrogenase and its effect on fermentation of xylose and lignocellulosic hydrolysate. Appl. Environ. Microbiol. 67:4249-4255. [PubMed] 33. Kötter, P., and M. Ciriacy. 1993. Xylose fermentation by Saccharomyces cerevisiaeSaccharomyces cerevisiae. Appl. Microbiol. Biotechnol. 38:776-783. 34. Krampe, S., O. Stamm, C. P. Hollenberg, and E. Boles. 1998. Catabolite inactivation of the high-affinity hexose transporters Hxt6Hxt6 and Hxt7Hxt7 of Saccharomyces cerevisiaeSaccharomyces cerevisiae occurs in the vacuole after internalization by endocytosis. FEBS Lett. 441:343-347. [PubMed] 35. Kurtzman, C. P., and J. W. Fell (ed.). 1998. The yeasts: a taxonomic study, 4th ed. Elsevier Science, Amsterdam, The Netherlands. 36. Kuyper, M., H. R. Harhangi, A. K. Stave, A. A. Winkler, M. S. Jetten, W. T. de Laat, J. J. den Ridder, H. J. Op den Camp, J. P. van Dijken, and J. T. Pronk. 2003. High-level functional expression of a fungal xylose isomerase: the key to efficient ethanolic fermentation of xylose by Saccharomyces cerevisiaeSaccharomyces cerevisiae? FEMS Yeast Res. 4:69-78. [PubMed] 37. Lascaris, R., H. J. Bussemaker, A. Boorsma, M. Piper, H. van der Spek, L. Grivell, and J. Blom. 2003. Hap4p overexpression in glucose-grown Saccharomyces cerevisiaeSaccharomyces cerevisiae induces cells to enter a novel metabolic state. Genome Biol. 4:R3. [PubMed] 38. Maleszka, R., and H. Schneider. 1984. Involvement of oxygen and mitochondrial function in the metabolism of d-xylulose by Saccharomyces cerevisiaeSaccharomyces cerevisiae. Arch. Biochem. Biophys. 228:22-30. [PubMed] 39. Neirinck, L. G., R. Maleszka, and H. Schneider. 1984. The requirement of oxygen for incorporation of carbon from d-xylose and d-glucose by Pachysolen tannophilusPachysolen tannophilus. Arch. Biochem. Biophys. 228:13-21. [PubMed] 40. Nissen, T. L., C. W. Hamann, M. C. Kielland-Brandt, J. Nielsen, and J. Villadsen. 2000. Anaerobic and aerobic batch cultivations of Saccharomyces cerevisiaeSaccharomyces cerevisiae mutants impaired in glycerol synthesis. Yeast 16:463-474. [PubMed] 41. Olesen, J., S. Hahn, and L. Guarente. 1987. Yeast HAP2 and HAP3 activators both bind to the CYC1CYC1 upstream activation site, UAS2UAS2, in an interdependent manner. Cell 51:953-961. [PubMed] 42. Ostergaard, S., L. Olsson, M. Johnston, and J. Nielsen. 2000. Increasing galactose consumption by Saccharomyces cerevisiaeSaccharomyces cerevisiae through metabolic engineering of the GALGAL gene regulatory network. Nat. Biotechnol. 18:1283-1286. [PubMed] 43. Passoth, V., M. Cohn, B. Schafer, B. Hahn-Hägerdal, and U. Klinner. 2003. Analysis of the hypoxia-induced ADH2ADH2 promoter of the respiratory yeast Pichia stipitisPichia stipitis reveals a new mechanism for sensing of oxygen limitation in yeast. Yeast 20:39-51. [PubMed] 44. Pettersen, R. C. 1984. The chemical composition of wood. Adv. Chem. Ser. 207: 57-126. 45. Reifenberger, E., E. Boles, and M. Ciriacy. 1997. Kinetic characterization of individual hexose transporters of Saccharomyces cerevisiaeSaccharomyces cerevisiae and their relation to the triggering mechanisms of glucose repression. Eur. J. Biochem. 245:324-333. [PubMed] 46. Ren, B., F. Robert, J. J. Wyrick, O. Aparicio, E. G. Jennings, I. Simon, J. Zeitlinger, J. Schreiber, N. Hannett, E. Kanin, T. L. Volkert, C. J. Wilson, S. P. Bell, and R. A. Young. 2000. Genome-wide location and function of DNA binding proteins. Science 290:2306-2309. [PubMed] 47. Schmidt, M. C., R. R. McCartney, X. Zhang, T. S. Tillman, H. Solimeo, S. Wolfl, C. Almonte, and S. C. Watkins. 1999. Std1 and Mth1 proteins interact with the glucose sensors to control glucose-regulated gene expression in Saccharomyces cerevisiaeSaccharomyces cerevisiae. Mol. Cell. Biol. 19:4561-4571. [PubMed] 48. Sedlak, M., H. J. Edenberg, and N. W. Ho. 2003. DNA microarray analysis of the expression of the genes encoding the major enzymes in ethanol production during glucose and xylose co-fermentation by metabolically engineered SaccharomycesSaccharomyces yeast. Enzyme Microb. Technol. 33:19-28. 49. Shi, N. Q., and T. W. Jeffries. 1998. Anaerobic growth and improved fermentation of Pichia stipitisPichia stipitis bearing a URA1URA1 gene from Saccharomyces cerevisiaeSaccharomyces cerevisiae. Appl. Microbiol. Biotechnol. 50:339-345. [PubMed] 50. Sonderegger, M., and U. Sauer. 2003. Evolutionary engineering of Saccharomyces cerevisiaeSaccharomyces cerevisiae for anaerobic growth on xylose. Appl. Environ. Microbiol. 69:1990-1998. [PubMed] 51. Tantirungkij, M., T. Izuishi, T. Seki, and T. Yoshida. 1994. Fed-batch fermentation of xylose by a fast-growing mutant of xylose-assimilating recombinant Saccharomyces cerevisiaeSaccharomyces cerevisiae. Appl. Microbiol. Biotechnol. 41:8-12. 52. ter Linde, J. J., H. Liang, R. W. Davis, H. Y. Steensma, J. P. van Dijken, and J. T. Pronk. 1999. Genome-wide transcriptional analysis of aerobic and anaerobic chemostat cultures of Saccharomyces cerevisiaeSaccharomyces cerevisiae. J. Bacteriol. 181:7409-7413. [PubMed] 53. Toivola, A., D. Yarrow, E. vanden Bosch, J. P. van Dijken, and W. A. Scheffers. 1984. Alcoholic fermentation by d-xylose by yeasts. Appl. Environ. Microbiol. 47:1221-1223. 54. Traff, K. L., R. R. O. Cordero, W. H. van Zyl, and B. Hahn-Hägerdal. 2001. Deletion of the GRE3GRE3 aldose reductase gene and its influence on xylose metabolism in recombinant strains of Saccharomyces cerevisiaeSaccharomyces cerevisiae expressing the xylAxylA and XKS1XKS1 genes. Appl. Environ. Microbiol. 67:5668-5674. [PubMed] 55. van Hoek, P., E. de Hulster, J. P. van Dijken, and J. T. Pronk. 2000. Fermentative capacity in high-cell-density fed-batch cultures of baker's yeast. Biotechnol. Bioeng. 68:517-523. [PubMed] 56. Verduyn, C., R. Van Kleef, J. Frank, H. Schreuder, J. P. Van Dijken, and W. A. Scheffers. 1985. Properties of the NAD(P)H-dependent xylose reductase from the xylose-fermenting yeast Pichia stipitisPichia stipitis. Biochem. J. 226:669-677. [PubMed] 57. von Mering, C., R. Krause, B. Snel, M. Cornell, S. G. Oliver, S. Fields, and P. Bork. 2002. Comparative assessment of large-scale data sets of protein-protein interactions. Nature 417:399-403. [PubMed] 58. Wahlbom, C. F., R. R. Cordero Otero, W. H. van Zyl, B. Hahn-Hägerdal, and L. J. Jonsson. 2003. Molecular analysis of a Saccharomyces cerevisiaeSaccharomyces cerevisiae mutant with improved ability to utilize xylose shows enhanced expression of proteins involved in transport, initial xylose metabolism, and the pentose phosphate pathway. Appl. Environ. Microbiol. 69:740-746. [PubMed] 59. Wang, P. Y., and H. Schneider. 1980. Growth of yeasts on d-xylulose. Can. J. Microbiol. 26:1165-1168. [PubMed]
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), glycerol (![[open diamond]](/corehtml/pmc/pmcents/diam.gif)
), xylose (![[open triangle]](/corehtml/pmc/pmcents/utri.gif)
), and xylitol (♦).