Two isogenic yeast strains were derived from the laboratory strain S. cerevisiae CEN.PK 113-7D. Single copies for the genes encoding CtXR in wild-type (strain BP000) or K274R-N276D double mutant form (strain BP10001) and XDH from Galactocandida mastotermitis (GmXDH) were inserted in the URA3-locus of the yeast genome together with an extra copy of the endogenous XK gene (Table 1). Both strains grew aerobically on xylose with nearly identical specific growth rates of about 0.07 h^-1. Their specific rates of growth and substrate consumption during aerobic and anaerobic conversion of glucose were also very similar. As expected, the reference strain S. cerevisiae CEN.PK 113-7D was unable to utilize xylose for aerobic growth or as fermentation substrate (data not shown). Table 2 summarizes specific activities of XR, XDH, and XK in cell extracts of BP000 and BP10001 cultivated aerobically in mineral medium containing 20 g/L of each glucose and xylose. However, xylose could be omitted from the medium without any effect on the specific activity of each of the three enzymes. For reasons we do not understand, BP10001 showed a significantly, about 1.8-fold higher level of XR activity than BP000, irrespective of various growth conditions and times of cell harvest used. The specific activity of XK was also higher (≈ 40%) in BP10001 than in BP000. The levels of XDH activity were comparable in the two strains. Cell extracts prepared by using Y-PER contained 1.4-fold higher specific XR activity than others obtained by disrupting exactly comparable cell material in a French Press. While the result is explicable on account of XR activity enhancement by the detergents present in Y-PER (data not shown; see ref. 42 for the effect of non-ionic detergents on activity and stability of CtXR), it also provides a note of caution regarding the comparison of enzyme activities that are based on different methods of yeast cell disruption.

Figure 2 compares XR activities of BP000 and BP10001 recorded at three concentrations of NADH and NADPH. The relative decrease in enzymatic rate in response to lowering the level of NADH from 350 μM to 7 μM was similar in the two strains. By contrast, the drop in activity caused by the same change in the concentration of NADPH was much more significant in BP10001 than in BP000. These results are in excellent agreement with expectations from the K_m values of purified wild-type (NADH: 38 μM; NADPH: 3 μM) and K274R-N276D (NADH: 41 μM; NADPH: 128 μM) 40. They also serve to verify functional expression of the double mutant in BP10001.

Batch conversions of xylose by glucose-grown resting cells of BP000 and BP10001 were carried out under oxygen-limited reaction conditions ([O₂] ≤ 20 μM) in shake flasks using a mineral medium that contained 20 g/L sugar. Typical fermentation time courses are shown in Figure 3 and parameters derived from their analysis are summarized in Table 3. No biomass was formed under these conditions. In a carbon balance calculated from the data in Figure 3 whereby CO₂ was inferred from the ethanol and acetate values, only ≤ 7% of the carbon from xylose remained unaccounted for. In comparison with the reference strain BP000, the XR double mutant strain BP10001 showed 40% enhanced ethanol yield. Its production of xylitol and glycerol was decreased by 53% and 30%, respectively. The yield of acetate was generally low in both strains, however, enhanced by about 50% in BP10001.

To verify the results of shake flask experiments under well controlled fermentation conditions where in particular the concentration of dissolved oxygen was monitored continuously, we compared anaerobic conversions of xylose (20 g/L) by BP10001 and BP000 carried out in a Braun Biostat bioreactor. Results are summarized in Figure 4 and Table 3. For both strains, the physiological parameters measured in the bioreactor were in good agreement with the ones obtained in shake flask. The glycerol yield was an exception as bioreactor experiments gave significantly lower values in this case. Likewise, the acetate yield for strain BP10001 was lower in bioreactor compared to shake flask cultivations and identical to the corresponding acetate yield for the control strain (0.019 g/g). Therefore, positive effects in the XR double mutant strain on xylose fermentation in shake flask could be scaled up fully to the laboratory bioreactor.

Biochemical constraints dictate that anaerobic conversion of xylose into ethanol is possible only when XR and XDH have matching coenzyme specificities 192143. The xylose pathway from Pichia stipitis which has served as point of departure for the construction of numerous xylose-fermenting strains of S. cerevisiae 46 does not fulfill this requirement well. Its XDH is strictly specific for NAD⁺ 44 while the XR strongly prefers NADPH over NADH 4546. Using known natural enzymes, the assembly of a chimeric pathway in which XR and XDH show exactly comparable utilization of NADP(H) and NAD(H) appears to be currently out of reach.

Protein engineering has therefore been pursued to make the coenzyme specificity of XR or XDH better compatible with that of the corresponding partner enzyme of the xylose pathway. Following the early studies by Metzger and Hollenberg 47, Makino and coworkers succeeded in creating a NADP(H)-dependent version of P. stipitis XDH through rational design 32. A notable feature of the best improved multiple mutant of XDH was a catalytic efficiency for the NADP⁺-dependent reaction that exceeded about 3.8-fold the corresponding efficiency of the wild-type using NAD⁺. While XDH from yeast and fungal sources is typically a Zn²⁺-dependent enzyme evolutionary related to medium-chain dehydrogenases/reductases 4849, bacterial polyol dehydrogenases possessing activity with xylitol do not use an active-site metal in catalysis and are found with the short-chain dehydrogenase/reductase superfamily of proteins 50. Ehrensberger and Wilson 51 determined a 1.9 Å crystal structure of XDH from Gluconobacter oxidans based on which they were able to convert the NAD⁺-dependent wild-type enzyme into a strictly NADP⁺-specific variant that had retained about 14% of the original catalytic efficiency for oxidation of xylitol.

Successful creation of a highly active XR mutant featuring a substantially lower preference for NADPH than the wild-type enzyme has strongly benefited from crystal structures of the enzyme from C. tenuis bound with NADP(H) 52 and NAD(H) 53. Some of the mutations found to be useful in CtXR 40 were later also introduced at homologous positions of the amino acid sequence of XR from P. stipitis 282954 (see later). Selection of the K274R-N276D doubly mutated CtXR for the in vivo experiments reported herein was based on a detailed steady-state kinetic characterization of a series of single and multiple-site variants of CtXR 40 and included analysis of mixed coenzyme utilization in the presence of physiological concentrations of NADPH and NADH 41. The double mutant eliminates the 33-fold preference of the wild-type for reaction with NADPH; however, it is clearly not a perfectly NADH-dependent enzyme. With the desired application for xylose fermentation in mind, it was important to also consider the possible effect of the mutated XR on the fluxional efficiency of the xylose pathway. The K274R-N276D double mutant was expected from its kinetic parameters to substitute the wild-type enzyme in the NAD(H)-dependent conversion of xylose without introducing an extra kinetic bottleneck.

The discussion will focus on physiological effects observed in stable xylose-fermenting strains of S. cerevisiae where the relevant genes were integrated into the yeast genome. Note, however, that preliminary reports have been published in which xylose fermentation by yeast strains expressing mutated P. stipitis XR or XDH from multi-copy plasmid vectors was investigated. They support the general idea that enhanced recycling of NADH 2829 or NADPH 3031 in the XR-XDH pathway helps decreasing xylitol formation and can eventually increase the ethanol yield. However, two independent studies, in which exactly the same mutants of P. stipitis XDH were examined, reached opposite conclusions regarding the effect on ethanol yield resulting from the usage of NADP⁺ instead of NAD⁺ in the XDH step 3031. These results emphasize the possible ambiguity in tracing back changes in strain physiology to the modification of the cosubstrate specificity of XR or XDH.

Therefore, the relevant phenotypes of the two isogenic yeast strains constructed in this work were carefully analyzed. Gene expression under control of the TDH3 promoter yielded levels of specific activity for XR (utilizing NADH), XDH, and XK that were about half those obtained by other groups who used the phosphoglycerate kinase 1 promoter for expressing the genes of the Pichia stipitis xylose pathway along with the endogenous XK gene 175556. (The comparison is relevant because purified CtXR 42 and GmXDH 57 display similar specific activities as the corresponding P. stipitis enzymes 444546.) The observed ratio of the specific activities of XR-NADH, XDH, and XK was 1: ≈5–7: ≈10 and lies within the window of operation recommended by Hahn-Hägerdal and co-workers 5558.

We were concerned about the difference in specific XR and XK activities found in strains BP000 and BP10001 that was substantially larger than expected from the estimated experimental error of 15 – 20% for the entire procedure of cell disruption and activity measurement. A gene copy number effect can be ruled out considering that (1) chromosomal integration of the three overexpressed genes occurred in a single step; and (2) unlike XR and XK, the specific activity of XDH was identical in both strains. However, for the purpose of strain comparison for xylose fermentation it may be noted that the specific uptake rates for the xylose substrate were very similar in BP000 and BP10001. We therefore regarded the two yeast strains as a suitable system for examining metabolic consequences resulting from the change in XR coenzyme specificity. The unknown source of variation in the specific enzyme activities was not further pursued.

The 52% decrease in xylitol yield resulting from the genetic replacement of wild-type CtXR by the K274R-N276D double mutant is quite significant in comparison to the success other metabolic engineering strategies have had in suppressing xylitol formation [for comprehensive reviews, see 12345], not only in terms of the magnitude of the effect but also because it was accompanied by similar changes in ethanol yield (42% increase) and glycerol yield (57% decrease). The acetate yield in bioreactor cultivations of the two strains was not affected within limits of the experimental error. Therefore, alteration of XR coenzyme specificity appears to have caused a global metabolic response, which contributes to a comprehensive improvement of the distribution of fermentation products.

It is interesting to bring into comparison these data with results of a detailed study by Jeppson et al. 56 who examined the effect of substituting wild-type XR from P. stipitis by a Lys²⁷⁰→Met mutant thereof, which according to studies of Lee and co-workers 59 exhibits a 17-fold higher K_m for NADPH than the native enzyme. The analogous site-directed replacement in CtXR, Lys²⁷⁴→Met, caused improvement of the coenzyme selectivity, NADPH compared to NADH, from a value of 33 in the wild-type enzyme to 5.5 in the mutant 40. However, it was also accompanied by a more substantial, 20-fold decrease in catalytic efficiency for the NADH-dependent reduction of xylose 40.

Despite the expected strong impairment of XR physiological function resulting from the mutation Lys²⁷⁰→Met 59, the yeast strain harboring a single gene copy for P. stipitis mutant XR consumed xylose in batch fermentations as fast as the isogenic control strain that contained native XR, and it produced less xylitol (0.17 vs. 0.29; 42% decrease) and more ethanol (0.36 vs. 0.31; 16% increase) 56. Formation of acetate and glycerol was, however, enhanced by about 40% in the mutant XR strain under these conditions. Interestingly, the effect of altered cosubstrate specificity of P. stipitis XR on ethanol yield was not clearly visible in strains that harbored two copies of the respective XR gene and hence consumed xylose about 1.5-fold faster than the corresponding single-copy strains.

In a continuous culture that used a mixed sugar substrate (10 g/L glucose, 10 g/L xylose), the strain harboring a single gene copy for the K270M mutant produced 8% more ethanol (0.40 g/g) and 41% less xylitol than the corresponding control strain. It was suggested from results of metabolic flux analysis that xylose conversion by the K270M mutant took place exclusively via NADH-dependent reaction while the wild-type form of P. stipitis XR showed balanced utilization of NADH and NADPH under these conditions (see later). Unfortunately, significant differences in physiological parameters for the native XR strains BP000 (Y_EtOH/xylose = 0.24; q_xylose = 0.06 h^-1, where Y is a yield coefficient and q is the specific uptake rate) and TMB3001 (Y_EtOH/xylose = 0.31; q_xylose = 0.145 h^-1 56) set a limit to the quantitative evaluation of the possible benefit, particularly on Y_EtOH/xylose, originating from the use of the K274R-N276D double mutant of CtXR (this work) compared to the K270M mutant of the P. stipitis enzyme 56.

Notwithstanding, if we assume that quantitative information about XR performance under in vivo conditions can be gleaned from the results of relevant in vitro assays 4041, the CtXR double mutant is expected to be a much superior catalyst with regard to both coenzyme selectivity and efficiency. Unfortunately, the large preference for NADPH seen with isolated preparations of native P. stipitis XR 4546 is very difficult to reconcile with the suggestion from metabolic flux analysis that a very substantial fraction of xylose (≈ 50%) is consumed by the enzyme in vivo via the NADH-dependent pathway 5660. Therefore, while further systematic integration of XR protein engineering into the development of novel xylose-fermenting strains of S. cerevisiae would seem to be a promising approach, it also requires that the apparent conflict in findings for in vitro and in vivo experiments be sorted out in future studies.

Escherichia coli strain TOP10 (Invitrogen, Carlsbad, CA, USA) was used as bacterial host for subcloning. Saccharomyces cerevisiae strain CEN.PK 113-7D (MATαMAL2-8c SUC2) was used for the isolation of yeast genomic DNA and as reference. Recombinant yeast strains were derived from uracil-deficient S. cerevisiae strain CEN.PK 113-5D. Plasmids pET11-CtXRWt 61 and pET11-CtXRDm 40 carry the genes encoding native and K274R-N276D double mutant forms of XR from Candida tenuis CBS4435, respectively. Plasmid pBTac1 62 carries the gene encoding XDH from Galactocandida mastotermitis. Construction of gene cassettes for expression in S. cerevisiae was performed using plasmid pRS416GPD 63. Yeast integrating vector YIp5 (DSMZ, Braunschweig, Germany) 40 was used for chromosomal insertion of the respective gene cassette.

Bacterial transformants were selected on Luria-Bertani medium agar plates supplemented with 112 mg/L ampicillin. Prior to transformation, yeast cells were grown in YPD medium. Transformants were selected on yeast synthetic complete media agar plates prepared from Yeast Nitrogen Base (Sigma, St. Louis, MO, USA) that contained Yeast Synthetic Drop-out Medium Supplements (Sigma) lacking uracil. Xylose fermentations in shake-flask and bioreactor cultivations were performed using a defined mineral medium containing vitamins and trace elements 56. The medium was supplemented with 0.01 g/L ergosterol, 0.42 g/L Tween 80 (dissolved in boiling 96 vol% ethanol), and 100 mM sodium citrate buffer, pH 5.5.

Restriction enzymes were from MBI Fermentas (St. Leon-Roth, Germany) or New England Biolabs (Beverly, MA, USA). Pfu DNA polymerase was from Promega (Madison, WI, USA). QIAprep Spin Miniprep Kit from Qiagen (Quiagen GmBH, Hilden, Germany) was used for plasmid preparation, and QIAquick Gel Extraction Kit was used for DNA extraction from agarose. Genomic DNA was isolated with the DNEasy Tissue Kit from Quiagen. Standard techniques of recombinant DNA technology and molecular biology were used.

In a first step, the promoterless genes for native or K274R-N276D CtXR, GmXDH, and the endogenous yeast XK1 were amplified from pET11-CtXRWt or pET11-CtXRDm, pBTac1, and genomic S. cerevisiae DNA, respectively. Polymerase chain reactions were performed using forward and reverse oligonucleotide primers whose 5'-ends contained a BamHI and SalI restriction site, respectively (see Table 4). Amplification products were digested with BamHI and SalI and inserted into the multiple cloning site of pRS416GPD, situated between the TDH3, formerly glyceraldehyde 3-phosphate dehydrogenase (GPD) promoter and the cytochrome-c-oxidase (CYC1) terminator. Gene cassettes were constructed where each of the target genes (XRWt, XRDm, XDH, and XK) was integrated separately between a TDH3 promoter and CYC1 terminator. Correct insertion was verified by sequencing. In a second step, the gene cassettes were amplified by PCR using oligonucleotide primers containing restriction sites at their respective 5'-end that are unique for YIp5 (see Table 4, Figure 5). The XK gene cassette was cloned into the AatII site, resulting in vector YXKS1. Third, the XDH gene cassette was inserted into the ClaI site of YXKS1, resulting in YGmXDH/XKS1. Fourth and finally, the gene cassette for either XRWt or XRDm was cloned into the EcoRI site of YGmXDH/XKS1, resulting in YCtXRWt/GmXDH/XKS1 and YCtXRDm/GmXDH/XKS1. Correct orientation of the inserted gene cassettes was verified after each step of integration using PCR screening with a pair of oligonucleotide primers matching a sequence upstream of the cloning site in the target vector and a sequence of the inserted gene.

Transformation of plasmids into Top10 competent cells was done by electroporation. Yeast integrating plasmids YCtXRWt/GmXDH/XKS1 and YCtXRDm/GmXDH/XKS1 were cleaved by SdaI within the URA3 gene. The linearized vectors were transformed into S. cerevisiae CEN.PK 113-5D using the lithium acetate method 64, resulting in the strains BP000 and BP10001 that express the gene encoding wild-type CtXR and the K274R-N276D double mutant thereof, respectively. Selected yeast strains were stored in 15% glycerol at -80°C.

Oxygen limitation during batch conversion of xylose by BP000 and BP10001 was achieved using 300-mL baffled shake flasks that were tightly closed with rubber stoppers. Two glass tubes were inserted in the stopper, one with a valve for purging with nitrogen and another containing a narrow slit at its closed far end which served as gas outlet. A magnetic stirrer bar (3 cm in diameter) was added to each shake flask. A fluorescence-based fiber-optic sensor (PreSens GmbH, Regensburg, Germany) was used to measure the concentration of dissolved O₂ in the medium each time when a sample was taken. The O₂ concentration never exceeded a value of 20 μM.

Yeast cells were grown overnight at 30°C and 110 rpm using a defined mineral medium that contained 20 g/L glucose. They were harvested by centrifugation (10 min; 4400 g) and after washing twice with 0.9% NaCl used for inoculation, to give a final optical density of ≈ 4. The working volume of each shake flask was 280 mL, and mineral medium containing 20 g/L xylose was used. The concentration of xylose at the start of the fermentation was increased in some cases to about 21 g/L as result of evaporation during the sterilisation. Note that reported data is always from measurements of the actual sugar concentrations. Shake flasks were purged with N₂ containing less than 5 ppm O₂ for 15 minutes before and 5 minutes after the inoculation. Further incubation of the sealed flasks was carried out at 30°C and 100 rpm using a Sartorius incubator. Care was taken that during withdrawing a sample (≈ 3 mL) from the shake flask, the biomass was homogeneously suspended. This was achieved by magnetic stirring and done under nitrogen purging. Work-up of samples and analytical procedures are described in a separate section, Analyses. Xylose fermentations were done in triplicate for each strain, and the results show mean values and the corresponding S.D. (Table 3, Figure 3)

A Braun Biostat C bioreactor equipped with two six-bladed disc impellers was used. The bioreactor had a working volume of 4 L. The ratio of impeller to reactor diameter was 0.4. Fermentations were carried out under conditions exactly comparable to the ones used for shake-flask experiments. The stirrer speed was set to a constant value of 200 rpm. The reactor was sparged with N₂ at a flow rate of 0.5 L/min. The pH was controlled at a value of 5.0 through automatic addition of 1 M NaOH.

Carbon balances for xylose fermentation in shake flasks are based on the assumption that 1 mole of CO₂ is formed per mole of ethanol and acetate. For carbon balances for fermentations in the bioreactor, CO₂ was calculated from the off gas analysis. Due to sparging with N₂, ethanol is evaporated from the bioreactor. The rate of ethanol evaporation was determined at a N₂ flow rate of 0.5 L/min, measuring by HPLC the decrease in the ethanol concentration as a function of time. Mineral medium lacking biomass was supplemented with 3 concentrations of ethanol between 1 and 4.5 g/L. Time-dependent loss of ethanol from this mixture could be described by a first-order decay function with a rate constant of 4.4 10^-3 h^-1. Reported values for the ethanol produced include the calculated evaporated alcohol.