- Open Access
Metabolic regulation analysis of an ethanologenic Escherichia coli strain based on RT-PCR and enzymatic activities
Biotechnology for Biofuelsvolume 1, Article number: 8 (2008)
A metabolic regulation study was performed, based upon measurements of enzymatic activities, fermentation performance, and RT-PCR analysis of pathways related to central carbon metabolism, in an ethanologenic Escherichia coli strain (CCE14) derived from lineage C. In comparison with previous engineered strains, this E coli derivative has a higher ethanol production rate in mineral medium, as a result of the elevated heterologous expression of the chromosomally integrated genes encoding PDC Zm and ADH Zm (pyruvate decarboxylase and alcohol dehydrogenase from Zymomonas mobilis). It is suggested that this behavior might be due to lineage differences between E. coli W and C.
This study demonstrated that the glycolytic flux is controlled, in this case, by reactions outside glycolysis, i.e., the fermentative pathways. Changes in ethanol production rate in this ethanologenic strain result in low organic acid production rates, and high glycolytic and ethanologenic fluxes, that correlate with enhanced transcription and enzymatic activity levels of PDC Zm and ADH Zm . Furthermore, a higher ethanol yield (90% of the theoretical) in glucose-mineral media was obtained with CCE14 in comparison with previous engineered E. coli strains, such as KO11, that produces a 70% yield under the same conditions.
Results suggest that a higher ethanol formation rate, caused by ahigher PDC Zm and ADH Zm activities induces a metabolic state that cells compensate through enhanced glucose transport, ATP synthesis, and NAD-NADH+H turnover rates. These results show that glycolytic enzymatic activities, present in E. coli W and C under fermentative conditions, are sufficient to contend with increases in glucose consumption and product formation rates.
Fermentative metabolism constitutes a fundamental cellular capacity for industrial biocatalysis. Endogenous organic compounds used by cells as terminal electron acceptors under oxygen deprivation are converted into biochemical products that are waste products for the cell, such as ethanol, lactate, acetate, succinate, formate and hydrogen, but represent valuable molecules to society . For example, renewable fuels from biomass, such as ethanol, constitute energy sources that preserve the environment since the carbon dioxide released from their combustion can be integrated into a photosynthetic cycle, which does not participate in a net carbon dioxide buildup into the atmosphere.
Metabolic engineering strategies have been used to modify microorganisms to convert all sugars arising from chemical-enzymatic hydrolysis of lignocellulose, such as xylose, arabinose, and glucose into ethanol. A wide variety of research approaches have been employed for this purpose; among the most effective attempts are the engineering of different Gram-negative bacteria, such as Escherichia coli [2–6], Klebsiella oxytoca [7–9] and Zymomonas mobilis [10, 11] as well as yeast, such as Saccharomyces cerevisiae [12–16]. One of the most successful strategies to develop ethanologenic bacteria was developed by Ingram and co-workers [2, 3, 6–8, 17]. In the case of E. coli, the W strain was engineered for ethanol production by integrating the pyruvate decarboxylase (pdc) and alcohol dehydrogenase (adhII) genes from Z. mobilis, under the control of the pflB promoter, to obtain strain KO11 [3, 17]. Expression from this promoter is high under anaerobic conditions [18, 19], and ethanologenic E. coli strains, such as KO11 and LY01 have shown to be efficient in the conversion of all sugars present in lignocellulosic hydrolysates into ethanol [20, 21].
Expression profiling is a powerful tool for analyzing gene transcription at a genomic scale. It can be used to compare global relative changes in gene expression that occur in response to an environmental stimulus or to compare the effects of genetic modifications on gene expression. This type of analysis can provide important information about cell physiology and has the potential to identify connections between regulatory or metabolic pathways not previously known [22, 23]. Since the physiological state and fermentation performance of a cell is dictated primarily at the protein level, transcription results should be complemented by determining specific enzyme activities to provide a better understanding of the observed phenomenon, considering that enzymatic and transcriptional regulation mechanisms are different .
Previous studies have shown that plasmid-encoded levels of Z. mobilis pyruvate decarboxylase (PDC Zm ) and alcohol dehydrogenase II (ADH Zm ) in E. coli correlate with the titer and the formation rate of ethanol [24, 21, 25]. Furthermore, the introduction of this heterologous pathway has several effects on E. coli physiology under fermentative conditions, i.e., increases its growth rate and glycolytic flux when cultivated in Luria Broth with xylose  or glucose . Gene array studies have also shown that several genes from the pentose phosphate and glycolytic pathways have statistically significant higher expression levels when ethanologenic E. coli (strain KO11) ferments xylose [26, 27].
The present study was conducted to understand the role that chromosomally integrated pdc Zm and adh Zm heterologous expression has on the physiology and metabolic performance of E. coli during glucose fermentation in mineral media. The regulation of metabolic pathways, related to central carbon metabolism and fermentation performance, was studied using mainly the measurements for both the enzymatic activities of the glycolytic and fermentative pathways, as well as transcript levels from genes coding for the enzymes involved in the glycolytic, pentose phosphate, and fermentative pathways. Glucose transporters and anaerobic regulators were also analyzed using transcriptome data. Evaluation was performed using wild type E. coli C as the reference strain, and a new ethanologenic strain derived from E. coli C, CCE14 (E. coli C: pflB::pdc adhB cat). Interestingly, strain CCE14 has ca. five-fold higher values of PDC Zm and ADH Zm enzymatic activities than strain KO11 (E. coli W: pflB::pdc adhB cat, Δfrd) [3, 17]. The results show that not only the specific ethanol rate, but also the glucose consumption rate (glycolytic flux) are increased as pyruvate decarboxylase and alcohol dehydrogenase transcripts and enzymatic activities are increased. Moreover, glycolytic flux is controlled by reactions outside glycolysis.
Results and discussion
Effect of PDCZm and ADHZm activity levels on fermentation performance
In comparison with the KO11 strain, PDC Zm and ADH Zm enzymatic specific activities were on average, 5 and 4-fold larger, respectively, in CCE14 during both exponential and stationary phases (Fig. 1). Even though the heterologous pathway was integrated into the chromosome of strains KO11 and CCE14 using the same method (see materials and methods section), strong differences were encountered between PDC Zm and ADH Zm enzymatic activities, as well as in transcript levels (as shown below). This behavior might be due to lineage differences between KO11 and CCE14. It is noteworthy that strain KO11 was submitted to high chloramphenicol pressure selection to increase ethanol productivity , in spite of this additional strategy, PDC Zm and ADH Zm activities were higher in CCE14, wich was not further selected on high chloramphenicol.
Fermentation performance in mineral medium with 40 g/L glucose is presented in Fig. 2. Fig. 2A–B shows results obtained for cell mass formation and glucose consumption. Table 2 summarizes rates obtained during the exponential and stationary phases. The growth rates of E. coli C, CCE14, and KO11 were similar. During exponential growth, specific glucose consumption rates of the two ethanologenic strains (KO11 and CCE14) were 28 and 34% higher, respectively, than that obtained for E. coli C, indicating that the glycolytic flux increased as a result of pdc Zm and adh Zm expressions. This behavior correlates well with previously reported results for KO11 fermenting xylose  or glucose  in Luria Broth, where the maximum sugar consumption rate was 50% higher for KO11 than for strain W. In spite of the fact that the growth rate was similar for the three strains, the maximum cell mass obtained at the onset of the stationary phase (after 20 hours of fermentation) was similar for KO11 and E. coli C, and lower for CCE14 (Table 2). These results, and data presented in Fig. 1, indicate that CCE14 directs more carbon to ethanol production than to biomass biosynthesis.
Fig 2C shows that no pyruvate was secreted by ethanologenic strains, but E. coli C produced a significant amount (> 3 g/L) of this metabolite during the stationary phase (Fig 2C). Furthermore, formate production by KO11 and E. coli C were similar, reaching up to 9 g/L when glucose was exhausted (Fig. 2D). However, formate production was lower than 2 g/L for CCE14. PDC Zm was originally selected by Ohta et al , largely because it has a very high affinity for pyruvate (Km for pyruvate 0.4 mM) [28, 29] in comparison with all competing fermentation enzymes . This fact and our results indicate that competition occurs at the pyruvate node level, and that higher levels of PDC Zm and ADH Zm apparently allow more efficient carbon channeling through the heterologous ethanol pathway.
Although glycolytic fluxes for CCE14 and KO11 were similar, the ethanol specific formation rate in the exponential phase (first 6 hours of fermentation elapsed time) was 21% higher for CCE14 as compared to KO11 (Table 3). During this phase, the ethanol formation rate in E. coli C was negligible (Fig. 2E), whereas formate (Fig. 2D) and acetate (Fig. 2F) were the main products. The increase in ethanol production rate was obtained at the expense of acid production (Table 3, Fig. 2). Pyruvate and lactate (Fig. 2C, 2G) were not produced during this phase in CCE14, whereas formate, acetate, (Fig. 2D, 2F), and succinate (Fig. 2H) production were significantly lower than for E. coli C and KO11. Balances for this phase indicate carbon recoveries very close to 100% for the three strains evaluated (Table 3). These results indicate that the glycolytic flux can be controlled by the efficient conversion of pyruvate into ethanol through the enzymatic activity levels of PDC Zm and ADH Zm in ethanologenic E. coli. It is hypothesized that other fermentative pathways that allow the efficient regeneration of NAD+ could have the same effect.
During the stationary phase, CCE14 produced ethanol 80% faster than KO11 (Table 4). Accordingly, specific enzyme activities of PDC Zm and ADH Zm were 6 and 4.7-fold higher for CCE14 (Fig. 1). Ethanol yields at 30 hours were 15, 70 and 90% of theoretical yield for E. coli C, KO11, and CCE14, respectively.
Metabolic regulation at transcript level
Transcript levels of 49 genes from the CCE14 strain were analyzed in the exponential growth phase and normalized for values obtained with E. coli C. Levels of pdc Zm and adh Zm were normalized with KO11 values and analyzed for both exponential and stationary phases. A Student' t-test with a p value of ≤ 0.05 was applied to each set of normalized values in order to determine statistical significant differences in expression levels.
Interestingly, the comparison of CCE14 and KO11 gave a direct relationship between increases in both pdc Zm and adh Zm transcript values (4.51 and 9.06-fold, respectively) (Fig. 3) and specific enzyme activity levels (5.1 and 3.8-fold, respectively) (Fig. 1). It has been reported that pdc Zm and adh Zm mRNA are more stable than other transcripts in Z. mobilis . A correlation was also found between CCE14 and KO11 during the stationary phase for transcripts (3.66-fold and 4.78-fold for pdc Zm and adh Zm , respectively) and specific enzyme activity levels (6-fold and 4.7-fold, respectively) (Fig. 1). Nevertheless, absolute values of the enzyme activity for these enzymes decreased around 50% during the stationary phase. The increase in specific ethanol formation rate (Table 4) correlated with higher transcript (Fig. 3) and specific enzyme activity (Fig. 1) levels for CCE14 in comparison to KO11. The requirements of higher PDC Zm enzymatic levels were demonstrated by Huerta-Beristain and co-workers . These authors reported that when PDC Zm activity increased 7-fold, using a multicopy plasmid, the yield of ethanol from glucose increased from 70 to 85%, whereas organic acid formation rates were reduced in the KO11 strain. Accordingly, results in Fig. 1 clearly show that increases in the specific activities of the enzymes participating in the ethanologenic pathway boost the carbon flow to ethanol in strain CCE14. These results also suggest that high levels of both enzymes are essential to increase the ethanol production rate. Pyruvate pools in ethanologenic E. coli are substantially reduced by high-level expression of these Z. mobilis genes, but cells adjust their metabolism to various levels along the glycolytic pathway to fulfill the carbon flux. Direct increments between transcripts and specific enzyme activities demonstrate the correct translation of pyruvate decarboxylase and alcohol dehydrogenase when they are over expressed.
Glucose transport and phosphorilation
Genes coding for proteins related to transport and regulation of glucose such as ptsG (1.98-fold), transcriptional repressor coding mlc (4.08-fold) [31, 32], high-affinity glucose transporters coding lamB (4.05-fold) and mglB (1.50-fold) , glucose kinase glk (2.58-fold), fruR (2.28-fold), and crp (2.02-fold) were more highly expressed in CCE14 than in E. coli C (Fig. 3). Specific glucose consumption rates (Table 2) and transport activities (Fig. 4) were on average 30 and 50% higher, respectively, for CCE14 in comparison with E. coli C. When glucose is phosphorylated in the course of transport, PTS proteins are dephosphorylated; unphosphorylated EIICBGlc causes the formation of the Mlc-EIICBGlc complex, derepressing the expression of target genes, such as mlc itself, as well as the pts operon . Therefore, higher levels of ptsG and mlc correlate with increases in IICBGlc (ptsG product) and MLC protein. The observed transcriptional pattern is consistent with a response that results in higher synthesis capacity for more PTS proteins necessary for glucose uptake.
On the other hand, wild type E. coli strains, growing on micromolar concentrations of glucose, synthetize galactose and maltodextrines as autoinducers derepressing the synthesis of the high-affinity glucose transport systems (MGLB and the LAMB maltoporin), which are responsible for glucose transport under these conditions . Analyses of gene expression response in wild type E. coli from glucose non-limiting to glucose-limiting growth conditions, in chemostat cultures, have demonstrated that several genes including mglB and lamB are upregulated . Furthermore, the crp transcript is higher when E. coli experience glucose limitation  and CRP regulates genes such as mglB, lamb, glk, and ptsG . Our results show that even though cultures were growing in large amounts of glucose (40 g/L) throughout the exponential phase (Fig. 2), transcription results suggest that CCE14 was sensing partial glucose limitation. This response might be due to increases in the fermentation and glycolytic rates that in turn will induce a response to scavenge sugar through transport activation of alternative glucose transporters. Interestingly, glk transcript levels were significantly higher in CCE14. This result suggests that besides the PTS system, glucose could also be transported by MGLB and LAMB and phosphorylated by GLK. The higher glk transcript is also related to an elicited response due to the over expression of heterologous genes as demonstrated by Arora and Pederson .
As mentioned earlier, fruR (2.28-fold) was more highly expressed in CCE14. FRUR (or CRA) is a key regulator controlling the balance between glycolysis and gluconeogenesis [38–40]. Many gluconeogenic genes are activated by FRUR, while glycolytic genes such as glk, pfkA, gapA, eno, and pykF are repressed. [41, 42]. However, none of the genes studied above was repressed. Probably FRUR was partially inactivated in the presence of glucose, because fructose-1-phosphate and fructose-1,6-bisphosphate bind to FRUR and inactivate its DNA-binding capacity [43, 44].
In general, only slight changes were detected in the transcription level of genes related to glycolysis. For instance, gapA (1.36-fold), fbaA (2.16-fold), and pgk (1.66-fold) transcript levels were higher in CCE14 strain than in E. coli C (Fig. 3). In E. coli, the gapA gene is transcribed from at least four promoters, three recognized by the RNA polymerase Eσ70 and one by the heat shock RNA polymerase Eσ32. This complex region of differentially regulated promoters allows the production of large amounts of gapA transcripts in a wide variety of environmental conditions . On the other hand, in γ-proteobacteria (E. coli, for example), the pgk and fbaA genes are cotranscriptionally expressed using two transcriptional promoters, though only one is required to get a strong production of PGK and FBA proteins in the presence of glucose . It has been proposed that when glucose is present in the growth medium, pts, gapA, and pgk genes are coordinately activated by a mechanism dependent upon the EIIGlc protein (coded by the ptsG gene) . Our results correlate with these facts, given the increases found in fbaA, pgk, and ptsG transcript levels.
Surprisingly, only the PGK enzymatic activity was higher (1.54-fold) in CCE14, whereas GAPDH activity was lower (0.64-fold) in this strain. As mentioned previously, it is possible that in the exponential phase, in spite of a higher transcript level of gapA, the low GAPDH activity could be related to a redox balance between GAPDH and higher ADH Zm and PDC Zm transcripts and enzymatic activities.
Several glycolytic genes showed no significant changes in the transcription level, and some of the transcripts and enzymatic activities did not show the same tendency. This behavior could be related to posttranscriptional regulation and RNA segmentation, leading to the production of individual mRNAs with selective stabilization. These processes allow the adaptation of gene expression to variations in environmental conditions, as has been observed in glycolytic gene expressions in B. subtilis [48, 49], Z. mobilis , and L. delbrueckii . Another explanation could be that enzyme levels are sufficient to carry out their catalytic role.
On the other hand, only the pgi transcript from CCE14 was lower than in the wild type strain. Likewise, the PGI enzymatic activity was slightly lower than that of E. coli C. Despite the importance of PGI in glycolysis, little information is available about the regulation of the pgi gene. However, due to the results in terms of glucose consumption and ethanol formation rate, the lower transcript and enzymatic activity does not cause any reduction in the glycolytic flux.
Entner-Doudoroff and pentose pathways
The zwf gene, that codes for glucose 6-P dehydrogenase, plays an important role in the control of carbon distribution at the glucose 6-phosphate node. It directs carbon flux through the oxidative branch of the pentose phosphate pathway (PPP) depending on NADP+ availability. In the CCE14 strain, the transcript level of zwf was not different to that of E. coli C (Fig. 3); however, ZWF specific enzyme activity was 7-fold higher in CCE14 (Fig. 4). Similarly, transcription of the gnd gene, which codes for phosphogluconate dehydrogenase, and one of the isoenzymes that codes for ribose-P isomerase (rpiB gene) were higher, 2.01 and 6.31-fold, respectively; while transcript of rpiA was lower, 0.71-fold. The isoenzimes transketolases (encoded by tktA and tktB genes) and transaldolase (encoded by talA and talB genes) interconnect glycolysis with the oxidative branch of PPP. Our results show that tktB and talA transcripts were lower, 0.46 and 0.56-fold, respectively, in CCE14; while tktA and talB were not different when compared to E. coli C. These results suggest that the pentose phosphate pathway is very flexible, and it is likely that overall catalytic rates are similar in the two strains tested.
Unexpectedly, genes edd that codes for 6-phosphogluconate dehydratase and eda which codes for 2-keto-3-deoxy-6-phosphogluconate aldolase in the Entner-Doudoroff pathway were more highly expressed, -2.17 and 2.24-fold, respectively, in CCE14 (Fig. 3). These results suggest that the Entner-Doudoroff pathway is functional, although it has been reported that for aerobic cultures with glucose the carbon flux through this route is not very high [52, 53]. In addition, ATP yield is lower through this pathway versus the Embden-Meyerhof pathway .
In the CCE14 strain, adhE (2.09-fold), fumB (2.13-fold), fumC (1.84-fold), frdABCD (2.84, 2.87, 2.38 2.45-fold), and pflD (3.43-fold) gene expressions were higher than in the wild type. It is known that frdABCD is induced under anaerobic conditions , though a recent study showed that this gene can be induced by glucose limitations .
It has been demonstrated that the fumB transcript is more abundant under anaerobic conditions, and that FNR is necessary as a transcriptional activator [57, 58]. In agreement with these reports, the transcription of fumB and the anaerobic regulator fnr (1.61-fold) were also more highly expressed in the CCE14 strain (Fig. 3). These results indicate that the pathways to produce succinate, formate, and ethanol (for native pathway) are active, although specific enzyme activity values of PFL and LDH and transcript levels of pflB and ldhA decreased in the exponential phase. It is important to mention that CCE14 produces formate and succinate in low concentrations. These results could indicate a competition phenomenon for pyruvate between PFL and PDC Zm . However, it is important to consider the disruption of routes to compete for the ethanol production in these conditions such as succinate and lactate pathways. We found that in cultures with high glucose concentrations (100 g/L), the production of succinate increases significantly in strain CCE14 (data no shown). This could be due to osmolarity problems or to a partial limitation of PYK enzyme causing PEP accumulation; hence, the carbon flux may be partially redirected towards succinate formation.
Metabolic regulation at the enzyme activity level
Enzyme activity levels for CCE14 strain were analyzed in exponential and stationary phases and normalized for values obtained with E. coli C (Fig. 4). Enzymatic levels for pdc Zm and adh Zm were normalized with KO11. A t-student test with a p value of ≤ 0.05 was applied to each set of normalized values to determine statistical differences in enzyme activity levels.
In the CCE14 strain, PTS and PGK enzymatic activities were higher, whereas TPI and PFL activities were lower during the exponential growth phase. These data correlate with the fact that ethanologenic strains consume glucose at a higher rate. In addition, increases in PGK activity suggest that the over expression of the genes coding for PDC Zm and ADH Zm modify the ATP/ADP balance. It is known that in aerobic conditions, a high ATP demand causes an increase in glycolytic flux in E. coli . For Lactococcus lactis, the control of glycolytic flux resides to a large extent in processes outside the pathway, such as ATP consuming reactions and glucose transport . As discussed above, the heterologous ethanologenic pathway increases glycolytic flux with the subsequent increases in ATP production and consumption. Therefore, it appears that cells tend to increase ATP formation through an increase in PGK synthesis; although no increase in PYK activity was found. ATP is also produced when acetate is formed; however, CCE14 does not produce acetate during the exponential phase. A decrease in PFL activity in CCE14 correlates with a strong reduction in formate production (Fig. 2D). On the other hand, the observed 50% reduction in the TPI specific enzyme activity does not reduce glycolytic flux. A large increase in ZWF specific activity was found, and was discussed above.
A comparison of enzymatic activity data between CCE14 and E coli C during the stationary phase, indicates higher values of PTS, FDP, GAPDH, PGK, and PYK for the ethanologenic strain. The LDH enzymatic activity was lower in CCE14. It is known that lactate dehydrogenase is allosterically activated by pyruvate . Lactate production was found only during the stationary phase of two cultures. Pyruvate formation in E. coli C correlates with lactate production (Fig. 2C–G), and lower levels of this metabolite in CCE14 correlate with a 40% lower LDH specific activity (Fig. 4). These results suggest that a higher ethanol formation rate, i.e., higher PDC Zm and ADH Zm specific activities originate higher rates of glucose transport, ATP synthesis, and NAD-NADH+H turnover.
A higher glycolytic flux in CCE14 results from increased chromosomal expression of pdc Zm and adh Zm genes and higher specific enzyme activities of heterologous PDC Zm and ADH Zm enzymes involved in ethanol formation. These results indicate that under the conditions used in this study, the glycolytic flux is controlled by reactions outside this pathway, that is, by the fermentative heterologous route. The metabolic adjustments carried out in the cell entail low organic acid production and an increase in the ethanol formation rate, as well as higher ethanol yield (90% of the theoretical) in glucose-mineral media when compared with previous engineered efficient strains, such as KO11 (70% of the theoretical yield). In spite of the higher PDC Zm and ADH Zm transcript and enzymatic activities in the CCE14 strain, the differences are mediated by higher glucose transport rates and an increase in the turnover rate of NAD-NADH+H+ and ATP.
Overall, these results also show that E. coli glycolytic enzymatic activities under fermentative conditions are sufficient to contend with increases in the rates of glucose consumption and higher transcript and enzymatic activities of the heterologous ethanol pathway. Also, the study provides the basis for the implementation of appropriate genetic modifications to increase the ethanol yield when mineral media is used; for instance, the disruption of succinate and lactate pathways that compete for ethanol production.
Bacterial strains, media and growth conditions
E. coli strains used in this work are listed in Table 1. With the purpose to have an ethanologenic strain with different PDC Zm and ADH Zm enzymatic levels, a new strain CCE14 was constructed integrating into the chromosome the pyruvate decarboxylase (pdc) and the alcohol dehydrogenase (adh) genes of Zymomonas mobilis under the control of the pfl native promoter. This chromosome integration was made with pLOI510 as described previously, . The vector pLOI510, was constructed to allow direct selection for the integration of pdc and adhB of Z. mobilis genes into the pfl region of the chromosome by using a DNA fragment which lacks a replicon . Transformants were screened for chloramphenicol resistance (20 μg/ml) and CO2 production in tubes, and subsequently tested for ethanol production in mini-fermentors with 20 g/l of glucose.
All stock cultures were stored at -70°C in Luria Broth (LB) medium  containing 40% glycerol. To develop inocula, cells were transferred twice on LB-agar plates supplemented with 20 g/L of glucose-chloramphenicol (20 μg/ml), and no chloramphenicol for E. coli C. Single colonies were transferred to overnight cultures in shake flasks (35°C, 120 rpm), containing glucose (20 g/L) in mineral M9-medium . M9-medium contains: 6 g/L Na2HPO4, 3 g/L KH2PO4, 1 g/L NH4Cl, 0.5 g/L NaCl. The following components were sterilized by filtration, and then added (per liter of final medium): 2 ml of 1 M MgSO47H2O, 1 mL of 0.1 M of CaCl2, 1 mL of 1 mg/mL thiamine-HCl. These cells were harvested in exponential growth phase by centrifugation and used to inoculate non-aerated mini-fermentors , containing 200 ml of M9-medium with 40 g/L of glucose. Starting OD600 was 0.1, chloramphenicol (0, 40 and 20 μg/ml) was included for strains C, KO11 and CCE14, (respectively), cells were cultivated at 35°C, 100 rpm, and the pH was maintained at 7 by the automatic addition of 2 N KOH. All cultures were carried out in triplicate.
Samples were periodically taken from cultures to measure optical density at 600 nm using a spectrophotometer (Beckman DU-70, Palo Alto, CA) and the dry cell weight was calculated using a previously determined conversion factor of 1 OD600 = 0.37 g/L. An HPLC system (600E quaternary bomb, 717 automatic injector, 2410 refractive index, and 996 photodiode array detectors, Waters, Milford, MA) and an Aminex HPX-87H column (300 × 7.8 mm; 9 μm) (Bio-Rad, Hercules, CA) were used to separate and quantify D-glucose, formate, acetate, succinate, and lactate concentrations. Running conditions were: mobile phase, 5 mM H2SO4, flow 0.5 ml/min, and temperature 50°C. Under these conditions glucose was detected by refractive index, and organic acids were identified by photodiode array at 210 nm. Ethanol was quantified by gas chromatography (Agilent 6850, Wilmington, D.E.), using 1-butanol as internal standard.
Preparation of cell extracts and enzymatic assays
Samples were taken at the mid-exponential and stationary phases. All operations were carried out at 4°C. 1 mL of cell culture was harvested by centrifugation at 10,000 × g for 10 min, washed twice with 1 mL of 100 mM Tris-HCl (pH 7.0) containing 20 mM KCl, 5 mM MnSO4, 2 mM DTT and 0.1 mM EDTA, and then suspended in 1 mL of the same buffer. Cells were disrupted by four sonication steps (15 s each) in an ultrasonic disrupter (Soniprep 150, UK). The cell debris was removed by centrifugation; 10 min at 10,000 × g. The resulting crude extracts were used immediately for determination of enzymatic activities and protein, or stored at -20°C.
Enzyme activities were measured spectrophotometrically at 340 nm in a thermostatically controlled (30°C) spectrophotometer (BioMate 5, ThermoSpectronic, NY). All compounds of the reaction mixtures were pipetted into 1 cm light path cuvettes, reactions were initiated by adding the cell extract or substrate to give a final volume of 1 mL. The millimolar extinction coefficient for NAD+, NADH, NADP+ and NADPH is 6.22 cm-1. mM-1.
The assay conditions for glucose:PEP phosphotransferase (PTS), 6-phosphofructosekinase (PFK), fructose-1,6-bisphosphatase (FDP), glucose phosphate isomerase (PGI), fructose bisphosphate aldolase (FDP aldolase), glyceldehyde-3-phosphate dehydrogenase (GAPDH), triose phosphate isomerase (TPI), 3-phosphoglycerate kinase (PGK), pyruvate kynase (PYK), 6-phosphogluconate dehydrogenase (ZWF), pyruvate-formate lyase (PFL), and lactate dehydrogenase (LDH) were measured based on the methods used by Peng et al . The assay conditions used for alcohol dehydrogenase (ADH Zm ) and pyruvate decarboxylase (PDC Zm ) were based on the methods reported by Conway et al . Phosphoglycerate mutase was measured based on the method of Maitra et al . Protein concentration was estimated by the Bradford method, , with bovine serum albumin used as the standard. Each assay was performed three times for the same culture, from three independent experiments. A t-student test with a p value of ≤ 0.05 was applied to each set of normalized values in order to determinate statistical differences in enzyme activity levels.
RNA extraction and cDNA synthesis
Total RNA extraction was performed using hot-phenol equilibrated with water, precipitated with 3 M sodium acetate and ethanol, and treated with DNase kit (DNA-free™, Ambion; . RNA integrity was tested by densitometry in 1.2% agarose gels. RNA quantification was performed by absorbance at 260/280 nm. cDNA was synthesized using RevertAid™ H First Strand cDNA Synthesis kit (Fermentas Inc.) and a mixture of specific DNA primers. The sequences of the primers used for cDNA synthesis were those reported by Flores et al , except for pdc Zm (5'-GACAAAGTTGCCGTCCTCGT and 5'-ATGGTAGCAACTGCGCCAC) and adh Zm (5'-TTACCCCGATGGTTTCCGT and 5'-TTCAAATGCGTGGGTCAGAG) genes. cDNA obtained in this way was used as template for RT-PCR assays. Reproducibility of this procedure was determined by performing two separate cDNA synthesis experiments from the RNA extracted for each strain. Similar results were obtained for the transcription of all genes that were measured.
Real-time PCR (RT-PCR) was performed with the ABI Prism 7000 Sequence Detection System (Perkin Elmer/Applied Biosystems, Foster City, CA), using the SYBR Green PCR Master Mix (Perkin Elmer/Applied Biosystems, Foster City, CA) and amplification conditions described by Flores et al . The primers for specific amplification were designated using the Primer Express software (Perkin Elmer/Applied Biosystems, Foster City, CA). The size of all amplimers was 101 bp. The final primer concentration, in a total volume of 15 μl, was 0.2 μM. Five nanograms of target cDNA for each gene was added to the reaction mixture. All experiments were performed in triplicate for each gene of each strain, obtaining very similar values. A non-template control reaction mixture was included for each gene. The quantification technique used to analyze data was the method described by Livak and Shmittgen . The data were normalized using the ihfB gene as an internal control (housekeeping gene). We detected the same expression level of this gene in all the strains in the conditions in which the bacteria were grown. For each analyzed gene in all strains, the transcription level of the wild type gene, considered as one, was used as the control to normalize the data. Data is reported as relative expression levels compared to the expression levels of E. coli C. A t-student test with a p value of ≤ 0.05 was applied to each set of normalized values in order to determinate statistical differences in expression levels.
Gottschalk G: Bacterial Metabolism. 2nd edition. Springer, New York Berlin Heidelberg; 1986:237.
Ingram LO, Conway T, Clark DP, Sewell GW, Preston JF: Genetic Engineering of Ethanol Production in Escherichia coli . Appl Environ Microbiol 1987, 53: 2420-2425.
Ohta K, Beall DS, Mejia JL, Shanmugam KT, Ingram LO: Genetic improvement of Escherichia coli for ethanol production: Chromosomal integration of Zymomonas mobilis genes encoding pyruvate decarboxylase and alcohol dehydrogenase II. Appl Environ Microbiol 1991, 57: 893-900.
Dien B, Hespell RB, Wyckoff HA, Bothast R: Fermentation of hexose and pentose sugars using a novel ethanologenic Escherichia coli strain. Enz Microbiol Technol 1998, 23: 366-371. 10.1016/S0141-0229(98)00064-7
Bothast RJ, Nichols NN, Dien BS: Fermentations with New Recombinant Organisms. Biotechnol Prog 1999, 15: 867-875. 10.1021/bp990087w
Martinez A, Grabar TB, Shanmugam KT, Yomano LP, York SW, Ingram LO: Low salt medium for lactate and ethanol production by recombinant Escherichia coli B. Biotechnol Lett 2007, 29: 397-404. 10.1007/s10529-006-9252-y
Ohta K, Beall DS, Mejia JL, Shanmugam KT, Ingram LO: Metabolic engineering of Klebsiella oxytoca strain M5A1 for ethanol production from xylose and glucose. Appl Environ Microbiol 1991, 57: 2810-2815.
Wood BE, Ingram LO: Ethanol production from cellobiose, amorphous cellulose, and crystalline cellulose by recombinant Klebsiella oxytoca containing chromosomally integrated Zymomonas mobilis genes for ethanol production and plasmids expressing thermostable cellulose genes from Clostidium thermocellum . Appl Environ Microbiol 1992, 58: 2103-2110.
Golias H, Dumsday GJ, Stanley GA, Pamment NB: Evaluation of a recombinant Klebsiella oxytoca strain for ethanol production from cellulose by simultaneous saccharification and fermentation: comparision with native cellobiose-utilising yeast strains and performance in co-culture with thermotolerant yeast and Zymomonas mobilis . J Biotechnol 2002, 96: 155-168. 10.1016/S0168-1656(02)00026-3
Zhang M, Eddy C, Deanda K, Finkelstein M, Picataggio S: Metabolic engineering of a Pentose Metabolism Pathway in Ethanologenic Zymomonas mobilis . Science 1995, 267: 240-243. 10.1126/science.267.5195.240
Deanda K, Zhang M, Eddy , Picataggio S: Development of an Arabinose-Fermenting Zymomonas mobilis strain by Metabolic Pathway Engineering. Appl Environ Microbiol 1996, 62: 4465-4470.
Ho NWY, Chen Z, Brainard AP: Genetically engineered Saccharomyces yeast capable of effective cofermentation of glucose and xylose. Appl Environ Microbiol 1998, 64: 1852-1859.
Becker J, Boles E: A Modified Saccharomyces cerevisiae Strain That Consumes L-Arabinose and Produces Ethanol. Appl Environ Microbiol 2003,69(7):4144-4150. 10.1128/AEM.69.7.4144-4150.2003
Jeffries TW, Jin YS: Metabolic engineering for improved fermentation of pentoses by yeast. Appl Microbiol Biotechnol 2004, 63: 495-509. 10.1007/s00253-003-1450-0
Hahn-Hägerdal B, Karhumaa K, Fonseca C, Spencer-Martins I, Gorwa-Grauslund MF: Towards industrial pentose-fermenting yeast strains. Appl Microbiol Biotechnol 2007, 74: 937-953. 10.1007/s00253-006-0827-2
van Maris AJA, Abbott DA, Bellissimi E, van den Brink J, Kuyper M, Luttik MAH, Wisselink HW, Scheffers WA, van Dijken JP, Pronk JT: Alcoholic fermentation of carbon sources in biomass hydrolysates by Saccharomyces cerevisiae : current status. Antonie van Leeuwenhoek 2006, 90: 391-418. 10.1007/s10482-006-9085-7
Jarboe LR, Grabar TB, Yomano LP, Shanmugam KT, Ingram LO: Development of Ethanologenic Bacteria. Adv Biochem Engin/Biotechnol 2007, 108: 237-261. [http://www.ncbi.nlm.nih.gov/pubmed/17665158?ordinalpos=5itool=EntrezSystem2.PEntrez.Pubmed.Pubmed_ResultsPanel.Pubmed_RVDocSum]
Sawers G, Bock A: Anaerobic regulation of pyruvate formate-lyase from Escherichia coli K-12. J Bacteriol 1988, 170: 5330-5336.
Sawers G, Bock A: Novel transcriptional control of the pyruvate formate-lyase gene: upstream regulatory sequences and multiple promoters regulate anaerobic expression. J Bacteriol 1989, 171: 2485-2498.
Yomano LP, York SW, Ingram LO: Isolation and characterization of ethanol-tolerant mutants of Escherichia coli KO11 for fuel ethanol production. J Ind Microbiol Biotechnol 1998, 20: 132-138. 10.1038/sj.jim.2900496
Martinez A, York SW, Yomano LP, Pineda VL, Davis FC, Shelton JC, Ingram LO: Biosynthetic burden and plasmid burden limit expression of chromosomally integrated heterologus genes ( pdc, adhB ) in Escherichia coli . Biotechnol Prog 1999, 15: 891-897. 10.1021/bp990103p
Kabir Md, Shimizu K: Gene expression patterns for metabolic pathway in pgi knockout Escherichia coli with and without phb genes based on RT-PCR. J Biotechnol 2003, 105: 11-31. 10.1016/S0168-1656(03)00170-6
Flores N, Escalante A, de Anda R, Báez-Viveros JL, Merino E, Franco B, Georgellis D, Gosset G, Bolívar F: New Insights into the Role of Sigma factor RpoS as Revealed in Escherichia coli Strains Lacking the Phosphoenolpyruvate:Carbohydrate Phosphotransferase System. J Mol Microbiol Biotechnol 2008, 14: 176-192. 10.1159/000109945
Ingram LO, Conway T: Expression of Different Levels of Ethanologenic Enzymes from Zymomonas mobilis in Recombinant Strains of Escherichia coli . Appl Environ Microbiol 1988, 54: 397-404.
Huerta-Beristain G, Utrilla J, Hernández-Chávez G, Bolívar F, Gosset G, Martinez A: Specific Ethanol Production Rate in Ethanologenic Escherichia coli strain KO11 Is Limited by Pyruvate Decarboxylase. J Mol Microbiol Biotechnol 2008, 15: 55-64. 10.1159/000111993
Tao H, Gonzalez R, Martinez A, Rodriguez M, Ingram LO, Preston JF, Shanmugam KT: Engineering a Homo-Ethanol Pathway in Escherichia coli : Increased Glycolytic Flux and Levels of Expression of Glycolitic Genes during Xylose Fermentation. J Bacteriol 2001, 183: 2979-2988. 10.1128/JB.183.10.2979-2988.2001
Gonzalez R, Tao H, Shanmugam KT, York SW, Ingram LO: Global Gene Expression Differences Associated with Changes in Glycolytic Flux and Growth Rate in Escherichia coli during the Fermentation of Glucose and Xylose. Biotechnol Prog 2002, 18: 6-20. 10.1021/bp010121i
Brau B, Sahm H: Cloning and expression of the structural gene for pyruvate decarboxylase of Zymomonas mobilis in Escherichia coli . Arch Microbiol 1986, 144: 296-301. 10.1007/BF00410966
Neale AD, Scopes RK, Wettenhall REH, Hoogenraad NJ: Pyruvate decarboxylase of Zymomonas mobilis : Isolation, properties and genetic expression in Escherichia coli . J Bacteriol 1987, 169: 1024-1028.
Mejia JP, Burnett ME, Haejung AN, Barnell WO, Keshav KF, Conway T, Ingram LO: Coordination of Expression of Zymomonas mobilis Glycolytic and Fermentative Enzymes: a Simple Hypothesis Based on mRNA Stability. J Bacteriol 1992, 174: 6438-6443.
Plumbridge J: Expression of ptsG , the gene for the major glucose PTS transporter in Escherichia coli , is repressed by Mlc and induced by growth on glucose. Mol Microbiol 1998, 29: 1053-1063. 10.1046/j.1365-2958.1998.00991.x
Nam TW, Cho SH, Shin D, Kim JH, Jeong JY, Lee JH, Roe JH, Peterkofsky A, Kang SO, Ryu S, Seok YJ: The Escherichia coli glucose transporter enzyme IICBGlcrecruits the global repressor Mlc. EMBO J 2001, 20: 491-498. 10.1093/emboj/20.3.491
Flores N, Flores S, Escalante A, de Anda R, Leal L, Malpica R, Georgelis D, Gosset G, Bolivar F: Adaptation for fast growth on glucose by differential expression of central carbon metabolism and gal regulon genes in an Escherichia coli strain lacking the phosphoenolpyruvate: carbohydrate phosphotransferase system. Metabol Eng 2005, 7: 70-87. [http://www.ncbi.nlm.nih.gov/pubmed/15781417?ordinalpos=18itool=EntrezSystem2.PEntrez.Pubmed.Pubmed_ResultsPanel.Pubmed_RVDocSum] 10.1016/j.ymben.2004.10.002
Hua Q, Yand C, Oshima T, Mori H, Shimizu K: Analysis of gene expression in Escherichia coli in response to changes of growth-limiting nutrient in chemostat cultures. Appl Environ Microbiol 2004, 70: 2354-66. 10.1128/AEM.70.4.2354-2366.2004
Postma PW, Lengeler JW, Jacobson GR: Phosphoenolpyruvate: Carbohydrate phosphotransferase systems. In Escherichia coli and Salmonella. Cellular and Molecular Biology. Edited by: Neidhardt FC. Washington, DC: American Society for Microbiology; 1996:1149-1174.
Báez-Viveros JL, Flores N, Juárez K, Castillo-España P, Bolivar F, Gosset G: Metabolic transcription analysis of engineered Escherichia coli strains that overproduce L-phenylalanine. Microb Cell Fact 2007, 6: 30. 10.1186/1475-2859-6-30
Arora KK, Pedersen PL: Glucokinase of Escherichia coli : Induction in Response to the Stress of Overexpressing Foreign Proteins. Arch Biochem Biophys 1995,319(2):574-578. 10.1006/abbi.1995.1333
Saier MH Jr: Cyclic AMP-independent catabolite repression in bacteria. FEMS Microbiol lett 1996, 138: 97-103. 10.1111/j.1574-6968.1996.tb08141.x
Saier MH Jr, Ramseier TM: Minireview. The catabolite repressor/activator (Cra) protein of enteric bacteria. J bacteriol 1996, 178: 3411-3417.
Crasnier-Mednansky M, Park MC, Studley WK, Saier MH Jr: Cra-mediated regulation of Escherichia coli adenylate cyclase. Microbiology 1997, 143: 785-792.
Chin AM, Feldheim DA, Saier MH Jr: Altered transcription patterns affecting several metabolic pathways in strains of Salmonella typhimurium which overexpress the fructose regulon. J Bacteriol 1989, 171: 2424-2434.
Ramseier TM, Bleding S, Michotey V, Feghali R, Saier MH Jr: The global regulatory protein FruR modulates the direction of carbon flow in Escherichia coli . Mol Microbiol 1995, 16: 1157-1169. 10.1111/j.1365-2958.1995.tb02339.x
Eisen MB, Spellman PT, Brown PO, Botstein D: Cluster analysis and display of genome-wide expression patterns. Proceedings of the National Academy of Sciences of the United States of America 1998, 95: 14863-14868. 10.1073/pnas.95.25.14863
Bledig SA, Ramseier TM, Saier MH Jr: FruR mediates catabolite activation of pyruvate kinase ( pykF ) gene expression in Escherichia coli . J Bacteriol 1996, 178: 280-283.
Charpentier B, Branlant C: The Escherichia coli gapA Gene Is Transcribed by the Vegetative RNA Polymerase Holoenzyme Eσ70and the Heat Shock RNA Polymerase Eσ32. J Bacteriol 1994, 176: 830-839.
Bardey V, Vallet C, Robas N, Charpentier B, Thouvenot B, Mougin A, Hajnsdorf E, Régnier P, Springer M, Bralant C: Characterization of the molecular mechanisms involved in the differential production of erythrose-4-phosphate dehydrogenase, 3-phosphoglycerate kinase and class II fructose-1,6-bisphosphate aldolase in Escherichia coli . Mol Microbiol 2005, 57: 1265-1287. 10.1111/j.1365-2958.2005.04762.x
Charpentier B, Bardey V, Robas N, Branlant C: The EIIGlcProtein Is Involved in Glucose-Mediated Activation of Escherichia coli gapA and gapB-pgk Transcription. J Bacteriol 1998, 180: 6473-6483. [http://www.ncbi.nlm.nih.gov/pubmed/9851989?ordinalpos=3itool=EntrezSystem2.PEntrez.Pubmed.Pubmed_ResultsPanel.Pubmed_RVDocSum]
Ludwing H, Homuth G, Schmalisch M, Dyka FM, Hecker M, Stulke J: Transcription of glycolytic genes and operons in Bacillus subtilis : evidence for the presence of multiple levels of control of the gapA operon. Mol Microbiol 2001, 41: 409-422. 10.1046/j.1365-2958.2001.02523.x
Doan T, Aymerich S: Regulation of glycolytic genes in Bacillus subtilis : binding of the repressor CggR to its single DNA target sequence is modulated by fructose-1,6-bisphosphate. Mol Microbiol 2003, 47: 1709-1721. 10.1046/j.1365-2958.2003.03404.x
Burchhardt G, Keshav KF, Yomano L, Ingram LO: Mutational Analysis of Segmental Stabilization of Transcripts from the Zymomonas mobilis gap-pgk Operon. J Biotechnol 1993, 175: 2327-2333. [http://jb.asm.org/cgi/reprint/175/8/2327?view=longpmid=8468293]
Branny P, de la Torre F, Garel JR: An operon encoding three glycolytic enzymes in Lactobacillus delbrueckii subsp. bulgaris : glyceraldehydes-3-phosphate dehydrogenase, phosphoglycerate kinase and triosephosphate isomerase. Microbiology 1998, 144: 905-914.
Flores S, Gosset G, Flores N, de Graaf AA, Bolívar F: Analysis of carbon metabolism in Escherichia coli strains with an inactive phosphotransferase system by 13C labeling and NMR spectroscopy. Metabol Eng 2002, 4: 124-137. [http://www.sciencedirect.com/science?_ob=ArticleURL_udi=B6WN3-45V802C-4_user=945819_rdoc=1_fmt=_orig=search_sort=dview=c_acct=C000048981_version=1_urlVersion=0_userid=945819md5=537d9456dc0f637cc3d453e1d7c6f11a] 10.1006/mben.2001.0209
Conway T: The Entner-Doudoroff pathway: history, physiology and molecular biology. FEMS Microbiol Rev 1992, 103: 1-28. [http://www.ncbi.nlm.nih.gov/pubmed/1389313?ordinalpos=11itool=EntrezSystem2.PEntrez.Pubmed.Pubmed_ResultsPanel.Pubmed_RVDocSum] 10.1111/j.1574-6968.1992.tb05822.x
Sprenger GA: Carbohydrate metabolism in Zymomonas mobilis : a catabolic highway with some scenic routes. FEMS Microbiol Lett 1996, 145: 301-307. 10.1111/j.1574-6968.1996.tb08593.x
Jones HM, Gunsalus RP: Transcription of the Escherichia coli Fumarate Reductase Genes ( frdABCD ) and Their Coordinate Regulation by Oxygen, Nitrate, and Fumarate. J Bacteriol 1985, 164: 1100-1109.
Franchini AG, Egli T: Global gene expression in Escherichia coli K-12 during short-term and long-term adaptation to glucose-limited continuos culture conditions. Microbiol 2006,152(Pt 7):2111-2127. [http://mic.sgmjournals.org/cgi/content/full/152/7/2111?view=longpmid=16804185] 10.1099/mic.0.28939-0
Tseng C, Yu C, Lin H, Chang C, Kuo J: Oxygen- and Growth Rate-Dependent Regulation of Escherichia coli Fumarase (FumA, FumB and FumC) Activity. J Bacteriol 2000,183(2):461-467. [http://www.ncbi.nlm.nih.gov/pubmed/11133938?ordinalpos=15itool=EntrezSystem2.PEntrez.Pubmed.Pubmed_ResultsPanel.Pubmed_RVDocSum] 10.1128/JB.183.2.461-467.2001
Partridge J, Scott C, Tang Y, Poole R, Green J: Escherichia coli Transcriptome Dynamics during the Transition from Anaerobic to Aerobic Conditions. J Biol Chem 2006, 281: 27806-27815. 10.1074/jbc.M603450200
Koebmann BJ, Westerhoff HV, Snoep JL, Nilsson D, Jensen PR: The glycolytic flux in Escherichia coli is controlled by the demand for ATP. J Bacteriol 2002, 184: 3909-3916. 10.1128/JB.184.14.3909-3916.2002
Papagianni M, Avramidis N, Filiousis G: Glycolysis and the regulation of glucose transport in Lactococcus lactis spp. lactis in batch and fed-batch culture. Microbial Cell Factories 2007, 6: 16. 10.1186/1475-2859-6-16
Tarmy EM, Kaplan NO: Kinetics of Escherichia coli B D-Lactate Dehydrogenase and Evidence for Pyruvate-controlled Change in Conformation. J Biological Chemistry 1968, 243: 2587-2596. [http://www.ncbi.nlm.nih.gov/pubmed/4297266?ordinalpos=1itool=EntrezSystem2.PEntrez.Pubmed.Pubmed_ResultsPanel.Pubmed_RVDocSum]
Maniatis T, Fritsch EF, Sambrook J: Molecular Cloning. In A Laboratory Manual. Cold Spring Harbor, Cold Spring Harbor Laboratory Press; 1982.
Beall DS, Ohta K, Ingram LO: Parametric studies of ethanol production from xylose and other sugars by recombinant Escherichia coli . Biotechnol Bioeng 1991, 38: 296-303. 10.1002/bit.260380311
Peng L, Shimizu K: Global metabolic regulation analysis for Escherichia coli K-12 based on protein expression by 2-dimensional electrophoresis and enzyme activity measurement. Appl Microbiol Biotechnol 2003, 61: 163-178.
Conway T, Osman YA, Donnan EM, Ingram LO: Promoter and nucleotide sequences of the Zymomonas mobilis pyruvate decarboxylase. J Bacteriol 1987, 169: 949-954.
Maitra PK, Lobo Z: A kinetic study of glycolytic enzyme synthesis in yeast. J Biol Chem 1971, 246: 475-488.
Bradford MM: A rapid and sensitive method for the quantitation of microgram quantitites of protein utilizing the principle of protein-dye binding. Analytical Biochemistry 1976, 72: 248-254. 10.1016/0003-2697(76)90527-3
Livak K, Shmittgen TD: Analysis of relative gene expression data using real-time quantitative PCR and the 2-ΔΔC T method. Methods 2001, 25: 402-408. 10.1006/meth.2001.1262
We thank Dr. Lonnie O. Ingram (University of Florida) for kindly providing strain KOll and pLOI510. We thank Mercedes Enzaldo, Ricardo Ciria and Manuel Hurtado for technical support. We thank Jonathan C. Moore (University of Florida) for proofreading of the manuscript. This work was supported by the Mexican Council of Science and Technology (CONACyT) grants: CONACyT-SAGARPA 2004-C01-224, CONACyT – Estado de Morelos MOR-2004-C02-048, CONACyT 44126 and PAPIIT-DGAPA-UNAM IN220908-3. Montserrat Orencio-Trejo held a scholarship from CONACyT.
The authors declare that they have no competing interests.
MOT Constructed the ethanologenic strain, carried out the kinetic, RT-PCR and enzyme characterization, the data analysis and drafted the manuscript. NF Participated in RT-PCR analysis and proofreading the manuscript. AE Participated in RT-PCR technique and proofreading the manuscript. GHC Participated in HPLC analysis. FB Reviewed and commented the manuscript. GG Reviewed and commented the manuscript. AM Conceived the study, designed and supervised the experiments, participated in results analysis and helped with manuscript preparation.