Effect of iclR and arcA knockouts on biomass formation and metabolic fluxes in Escherichia coli K12 and its implications on understanding the metabolism of Escherichia coliBL21 (DE3)
© Waegeman et al; licensee BioMed Central Ltd. 2011
Received: 13 September 2010
Accepted: 11 April 2011
Published: 11 April 2011
Gene expression is regulated through a complex interplay of different transcription factors (TFs) which can enhance or inhibit gene transcription. ArcA is a global regulator that regulates genes involved in different metabolic pathways, while IclR as a local regulator, controls the transcription of the glyoxylate pathway genes of the aceBAK operon. This study investigates the physiological and metabolic consequences of arcA and iclR deletions on E. coli K12 MG1655 under glucose abundant and limiting conditions and compares the results with the metabolic characteristics of E. coli BL21 (DE3).
The deletion of arcA and iclR results in an increase in the biomass yield both under glucose abundant and limiting conditions, approaching the maximum theoretical yield of 0.65 c-mole/c-mole glucose under glucose abundant conditions. This can be explained by the lower flux through several CO2 producing pathways in the E. coli K12 ΔarcAΔiclR double knockout strain. Due to iclR gene deletion, the glyoxylate pathway is activated resulting in a redirection of 30% of the isocitrate molecules directly to succinate and malate without CO2 production. Furthermore, a higher flux at the entrance of the TCA was noticed due to arcA gene deletion, resulting in a reduced production of acetate and less carbon loss. Under glucose limiting conditions the flux through the glyoxylate pathway is further increased in the ΔiclR knockout strain, but this effect was not observed in the double knockout strain. Also a striking correlation between the glyoxylate flux data and the isocitrate lyase activity was observed for almost all strains and under both growth conditions, illustrating the transcriptional control of this pathway. Finally, similar central metabolic fluxes were observed in E. coli K12 ΔarcA ΔiclR compared to the industrially relevant E. coli BL21 (DE3), especially with respect to the pentose pathway, the glyoxylate pathway, and the TCA fluxes. In addition, a comparison of the genome sequences of the two strains showed that BL21 possesses two mutations in the promoter region of iclR and rare codons are present in arcA implying a lower tRNA acceptance. Both phenomena presumably result in a reduced ArcA and IclR synthesis in BL21, which contributes to the similar physiology as observed in E. coli K12 ΔarcAΔiclR.
The deletion of arcA results in a decrease of repression on transcription of TCA cycle genes under glucose abundant conditions, without significantly affecting the glyoxylate pathway activity. IclR clearly represses transcription of glyoxylate pathway genes under glucose abundance, a condition in which Crp activation is absent. Under glucose limitation, Crp is responsible for the high glyoxylate flux, but IclR still represses transcription. Finally, in E. coli BL21 (DE3), ArcA and IclR are poorly expressed, explaining the similar fluxes observed compared to the ΔarcAΔiclR strain.
The genome of the bacterium Escherichia coli consists of 4.6 million base pairs and contains 4288 genes . If all genes would be transcribed simultaneously, the cell volume should be at least threefold higher to harbor all proteins produced. Furthermore, under specific environmental conditions, transcription of only a limited set of genes is necessary to ensure optimal growth. In order to control which genes are transcribed, transcription is controlled by the interplay of numerous regulators .
Transcriptional regulators or transcription factors (TFs) are proteins that bind to specific sequences of the DNA, i.e. promoters, and hereby facilitate or inhibit the binding of RNA polymerase (RNAP). A low RNAP affinity generally results in low gene expression, while a higher RNAP affinity corresponds with an increased gene expression. However, if the affinity is too strong, gene expression decreases again due to a too weak mobility of the RNAP [3–5].
Regulation of gene expression is very complex and transcriptional regulators can be subdivided into global and local regulators depending on the number of operons they control. Global regulators control a vast number of genes, which must be physically separated on the genome and belong to different metabolic pathways . Only seven global regulators are required to control the expression of 51% of all genes: ArcA, Crp, Fis, Fnr, Ihf, Lrp, and NarL. In contrast to global regulators, local regulators control only a few genes, e.g. 20% of all TFs control the expression of only one or two genes . The regulators investigated in this study are the global regulator ArcA and the local regulator IclR.
ArcA (anaerobic redox control) was first discovered in 1988 by Iuchi and Lin and the regulator seemed to have an inhibitory effect on expression of aerobic TCA cycle genes under anaerobic conditions . ArcA is the regulatory protein of the dual-component regulator ArcAB, in which the later discovered ArcB acts as sensory protein . Statistical analysis of gene expression data  showed that ArcA regulates the expression of a wide variety of genes involved in the biosynthesis of small and macromolecules, transport, carbon and energy metabolism, cell structure, etc. The regulatory activity of ArcA is dependent on the oxygen concentration in the environment and the most profound effects of arcA gene deletion are noticed under microaerobic conditions . In contrast, under anaerobic conditions Fnr (fumarate nitrate reductase) is the predominant redox sensing global regulator [12–14]. Recently however, it was discovered that also under aerobic conditions ArcA has an effect on central metabolic fluxes .
The second regulator investigated in this study, isocitrate lyase regulator (IclR), represses the expression of the aceBAK operon, which codes for the glyoxylate pathway enzymes isocitrate lyase (AceA), malate synthase (AceB), and isocitrate dehydrogenase kinase/phosphatase (AceK) . The last enzyme phosphorylates the TCA cycle enzyme isocitrate dehydrogenase (Icd), which results in a reduction of Icd activity and consequently in a reduction of the flux through the TCA cycle . When IclR levels are low or when IclR is inactivated, i.e. for cells growing on acetate [18–20], or in slow-growing glucose-utilizing cultures [21, 22], repression on glyoxylate genes is released and the glyoxylate pathway is activated.
Although the effect of single deletions of genes, coding for global regulators, on metabolism have been extensively studied [15, 23], their double knockouts have rarely been investigated. So far, in vivo only the effects of arcA-fnr , arcA-cra , and crp-fur  knockout combinations have been studied. Recently, two studies focused on the effect of the deletion of genes coding for a global regulator and a local regulator, i.e. cra-iclR and crp-iclR [26, 27], on gene expression and activities of key metabolic enzymes. However, the effect of the knockouts on the metabolic fluxes were not investigated.
This study investigates such a knockout combination and shows that the combined deletion of arcA and iclR has a profound effect on metabolism and redirects carbon fluxes in such a way that the biomass content increases remarkably both under glucose abundant and glucose limiting conditions as opposed to its parent strain E. coli K12 MG1655. Many of the observed characteristics in the double knockout strain are also ascribed to E. coli BL21 (DE3), which is why fluxes between these two strains were investigated as well.
Results and Discussion
Physiological effects of arcA and iclRdeletions
Average maximum growth rates (batch) and dilution rates (chemostat) of the different strains.
μ max (h-1)
D influent (h-1)
D effluent (h-1)
0.66 ± 0.02
0.099 ± 0.001
0.100 ± 0.001
0.60 ± 0.01
0.118 ± 0.001
0.120 ± 0.001
0.61 ± 0.02
0.085 ± 0.001
0.090 ± 0.001
0.44 ± 0.03
0.090 ± 0.001
0.093 ± 0.001
Under glucose abundant conditions (see Figure 1A), the following trends can be observed. Both the arcA and iclR knockout strains show an increased biomass yield. When combining these deletions (i.e. in ΔarcAΔiclR) the yield is further increased to 0.63 ± 0.01 c-mole/c-mole glucose, which approximates the theoretical biomass yield of 0.65 c-mole/c-mole glucose (assuming a P/O-ratio of 1.4) [28, 29]. The higher biomass yield is accompanied by a 70 and 16% reduction in acetate and CO2, respectively.
The results of the glucose limited cultures are shown in Figure 1B. The ΔarcAΔiclR strain exhibits an increased biomass yield compared to the wild type strain (0.52 ± 0.01 c-mole/c-mole vs. 0.46 ± 0.01 c-mole/c-mole), but the increment in biomass yield (i.e. 13%) is less distinct as observed under glucose abundant conditions (47%).
The increment in biomass yield is less pronounced under glucose limitation, because glucose limited cultures of the strain ΔarcAΔiclR show a decreased biomass yield while the wild type shows an increased biomass yield compared to if these strains are cultivated under glucose abundant conditions. This can be easily explained: under glucose abundance, the wild type strain converts 16% of the carbon source to acetate as a result of overflow metabolism . At a fixed, low growth rate and consequently under glucose limitation, the cell can easily cope with the delivered carbon and very little carbon is dissipated through formation of byproducts. However, energy losses also occur in continuous cultures because of the existence of futile cycles . In addition, as shown by Pirt and many others, an excessive fraction of the energy source is reserved for growth-independent maintenance, a factor which is relatively higher under glucose limitation [32–36]. For the wild type cultivated at a low growth rate (D = ±0.1 h-1), the absence of energy spilling by overflow metabolism compensates and even exceeds the energy spilling by futile cycling and the energy reserved for maintenance, explaining the higher biomass yield observed. In contrast, the ΔarcA ΔiclR strain does not show overflow metabolism under glucose abundance, and therefore the effects of energy loss by futile cycles and maintenance are more visible in this strain leading to a lower biomass yield under glucose limitation.
Activity of glyoxylate cycle enzymes
Relative activities of malate synthase and isocitrate lyase under glucose abundant (batch) and limiting (chemostat) conditions.
Isocitrate lyase activity
Malate synthase activity
1.00 ± 0.10
10.13 ± 1.43
1.00 ± 0.19
0.11 ± 0.03
0.33 ± 0.04
32.47 ± 3.61
0.36 ± 0.07
2.13 ± 0.39
5.69 ± 0.57
26.96 ± 3.06
1.38 ± 0.27
0.24 ± 0.04
6.39 ± 0.64
26.52 ± 2.78
0.48 ± 0.08
2.92 ± 0.52
The isocitrate lyase activity levels of the strains cultivated under glucose abundant conditions are rather low compared to those obtained under glucose limiting conditions. Remarkably, under glucose excess deletion of iclR results in an almost sixfold increase in the enzymes activity compared to the wild type. Deleting arcA as well (in the resulting ΔarcAΔiclR strain) did not evoke a significant increase in isocitrate lyase activity compared to the enzyme activity in the ΔiclR strain, which indicates that IclR is a stronger repressor of the aceBAK operon as opposed to ArcA under these conditions.
Under glucose limiting conditions, the wild type isocitrate lyase activity is enhanced 10 times compared to batch conditions, which is in accordance with previous proteome analysis of glucose limited cultures [37, 38] and enzyme activity levels [22, 38] under similar growth conditions. This is presumably due to different cAMP levels under glucose abundant and limiting conditions, since cAMP binding to Crp is necessary for regulatory activity of Crp.
Under high glucose levels, cAMP concentrations are low and the cAMP-Crp complex cannot be formed. Consequently, activation of transcription of glyoxylate pathway genes by Crp cannot occur. If crp is deleted from the genome (i.e. in a Δcrp strain), no major differences in transcript levels of aceA or aceB between a culture grown under high and low glucose levels should be noticed, which was confirmed by transcriptome analysis . Furthermore if Crp represses transcription of glyoxylate genes under high glucose levels as alleged in a few studies [25, 39], a difference in aceA and aceB transcript levels should be noticed between the wild type and the crp knockout strain under high glucose concentrations, which was not observed .
Under glucose limiting conditions however, cAMP levels rise and the cAMP-Crp complex is properly formed, enabling the functioning of the regulator. Now Crp binds the DNA, competes with the binding of the repressor IclR and hereby activates transcription. If under these low glucose concentrations Crp is absent (i.e. in a Δcrp strain), the activities of the enzymes involved in the glyoxylate shunt should drop, since IclR can now fully repress aceBAK transcription. This was confirmed by Nanchen et al. who studied the behavior of a Δcrp strain under glucose limitation . However, the transcription of glyxoylate genes is the result of the regulatory activity of multiple regulators and not only Crp. If the repressors IclR and ArcA are inactive, i.e. in the ΔiclR and the ΔarcA strain, isocitrate lyase levels are increased compared to the wild type (see Table 2).
The malate synthase activity in E. coli is the result of the activity of two isoenzymes, malate synthase A (gene: aceB) and G (gene: glcB) . Both genes are members of different operons and the corresponding enzymes are members of different pathways, i.e. malate synthase A is the second enzyme of the glyoxylate pathway, whereas malate synthase G acts in the glycolate pathway. Figure 3B depicts the transcriptional regulation of the glc operons.
The obtained malate synthase activities (see Table 2) are somewhat contra-intuitive. Since Crp is also an activator of the glcC operon , one expects similar activity levels for isocitrate lyase and malate synthase, which was not observed. Nonetheless, some conclusions can be derived from the data. ArcA represses both glcB and aceB expression, thus both enzyme activities should increase in the knockout strain (assuming that there is no translational regulation involved). This explains the twentyfold increment in malate synthase activity in the ΔarcA strain under glucose limiting conditions. Rather small differences are noticed between the wild type and the ΔiclR strain in both growth conditions, implying that IclR does not greatly affect malate synthase activity. Either IclR has a moderate influence on gene expression of malate synthase A, or post-translational effects are taking place, or the malate synthase activity is primarily the result of the malate synthase G activity (glcB), as IclR is not a regulator of the glc operons. If IclR has a limited influence on aceB expression, one expects a similar action on aceA as both genes are members of the same operon. Second, if the activity is heavily affected by post-translational events, one does not expect such great differences between the ΔarcA strain and the wild type or ArcA should have an influence on the post-translational process. Since the former phenomena were not observed, it is very likely that the malate synthase activity is predominantly the result of glcB expression. Other regulators of the glc operon, besides ArcA and Crp, are GlcC, IHF, and Fis (Figure 3B). The action of these other regulators can explain the results of the batch cultures. The activator IHF has limited activity in exponentially growing cells , but the regulation of the glc operon is even further complicated by the possibility of acetate cross-inducing the operon .
Because of the interference of the malate synthase G activity in the measurement of malate synthase activity, it can be concluded that the measurement of isocitrate lyase activity is a better indicator for glyoxylate pathway activity.
Glycogen and trehalose content
Glycogen content of the wild type and the double knockout strain under glucose abundant (batch) and glucose limiting (chemostat) conditions.
0.25 ± 0.26
0.50 ± 0.24
1.47 ± 0.19
1.29 ± 0.16
Considering the product yield and storage compound results, it can be concluded that the increase in biomass yield in the double knockout strain is primarily the result of the lower acetate and CO2 production under glucose abundant conditions and of the lower CO2 production under glucose limitation. Only a small and similar amount of the extra carbon is converted to storage molecules like glycogen under both growth conditions.
Effect of arcA and iclRknockouts on metabolic fluxes
Under glucose abundant conditions, deleting arcA results in a decrease of the OAA from PEP fraction, indicating that a higher fraction of OAA originates from the TCA cycle (OAA from TCA = 1 - OAA from PEP - OAA from glyoxylate). This phenomenon is also observed in the double knockout strain. Deletion of iclR results in an increase of the OAA from glyoxylate fraction from 0 to 23%. This effect is also retained in the double knockout strain ΔarcA ΔiclR. A third effect noticed in the double knockout strain is the significantly increased amount of serine originating from the Embden-Meyerhof-Parnas pathway (glycolysis) compared to the wild type (see Figure 4).
Under glucose limiting conditions a higher fraction of serine through EMP was observed for all strains as compared to the wild type under batch conditions. Furthermore the OAA from glyoxylate and the PEP from OAA fractions are increased compared to under glucose excess, implying the activation of the glyxylate cycle and gluconeogenesis. These fractions are even further increased in the ΔiclR strain which proves that also under glucose limiting conditions, IclR regulates the glyoxylate shunt, together with Crp and other regulators. In the double knockout strain the OAA from glyoxylate fraction decreases compared to the ΔiclR strain, which seems to be affected by the arcA deletion (see Figure 4). This is not expected as both IclR and ArcA are repressors of the pathway.
Under glucose abundant conditions (Figure 5A) the ΔarcA strain exhibits a significantly higher TCA flux as opposed to the wild type. This is the result of the omission of repression due to arcA deletion on transcription of almost all TCA cycle genes or operons: gltA, acnAB, icd, sucABCD, lpdA, sdhCDAB, fumAC, and mdh [10, 50–53] which was also observed by . This further demonstrates the regulatory action of ArcA under aerobic conditions, although its main action was considered to be under microaerobic growth conditions [13, 14]. The iclR single knockout strain exhibits similar glycolytic fluxes compared to the wild type, but at the PEP-pyruvate-oxaloacetate node fluxes are profoundly altered. Due to the iclR deletion, transcription of glyoxylate pathway genes is not longer inhibited. The flux data are in line with the isocitrate lyase activity measurements as shown in Table 2. In the ΔiclR and the ΔarcAΔiclR strain the activation of the glyxoylate pathway is linked to only a minor increase in the flux from oxaloacetate to PEP, implying that the PEP-glyxoylate cycle is not active under glucose excess. As a result, part of the carbon is channeled through the glyoxylate pathway, less CO2 is produced in the TCA cycle and the extra CO2 saved is not lost in the oxaloacetate to PEP reaction, contributing to the higher biomass yield observed in these strains. This corresponds with the lower CO2 yields of these strains in Figure 1A.
Under glucose limitation, relative fluxes around the PEP-pyruvate-oxaloacetate node are higher as opposed to under glucose excess. Not only the flux converting pyruvate to acetyl-CoA at the entrance of the TCA cycle is increased, but also the glyoxylate pathway is active and gluconeogenic fluxes from malate to pyruvate and from oxaloacetate to PEP are higher compared to under batch conditions. These reactions create the PEP-glyoxylate cycle. This novel metabolic cycle was identified quite recently  and functions as an alternative to the TCA cycle for the oxidation of carbohydrates. Similar to the TCA cycle, this pathway produces CO2, i.e. in the reaction from OAA to PEP. As a result of the simultaneous activity of the TCA cycle and the PEP-glyoxylate cycle, more glucose is oxidized to CO2 compared to batch cultures in order to produce energy and meet the higher maintenance demand . This is in accordance with the higher CO2 production and O2 consumption observed in glucose limited cultures (see Figure 1B vs 1A). Another effect observed between glucose limiting and abundant growth conditions is the reduced flux from 6-phosphogluconate to pentose-5-P by 6-phosphogluconate dehydrogenase (Gnd) for all strains in glucose limiting conditions (see Figure 5B vs 5A), which could be explained by the reduced transcription of gnd at lower growth rates [54–56].
Glyoxylate pathway flux data and regulation of the aceBAKoperon
The glyoxylate pathway flux data can also be used to investigate the interplay of different regulators on the aceBAK operon.
Under batch conditions, when Crp-cAMP levels are low and Crp cannot perform its activating role, no aceBAK transcription occurs and the glyoxylate pathway is inactive. However when the aceBAK repressor IclR is absent (i.e. in the ΔiclR strain), the glyoxylate pathway is active. This is illustrated by calculating the AceA/(AceA + Icd) flux ratio, which is much higher in the ΔiclR strain (32%) compared to the wild type (0%). This shows that Crp activation is not absolutely necessary for transcription. The absence of the repressor IclR is sufficient to obtain glyoxylate pathway activity. On the contrary, under glucose limitation, Crp-cAMP levels are high , the aceBAK transcription is enhanced and the glyoxylate bypass is active even in the presence of the repressor IclR. This is in line with the high value of the AceA/(AceA + Icd) flux ratio of the wild type (55%) compared to under batch conditions (0%). If under glucose limiting conditions iclR is inactivated, the AceA/(AceA + Icd) flux ratio increases even further to 63%. This clearly shows that both Crp and IclR regulate the aceBAK operon independently.
Under glucose abundant conditions, deleting arcA does not have a major effect on glyoxylate pathway fluxes (wild type vs. ΔarcA and ΔiclR vs. ΔarcAΔiclR), despite the fact that ArcA is a known repressor of the aceBAK operon . This is in stark contrast with the glyoxylate pathway fluxes under glucose limiting conditions. Here, arcA deletion reduces the bypass activity but only in a ΔiclR genetic environment. This is illustrated by the AceA/(AceA + Icd) flux ratio, which decreases from 55% in the wild type to 34% in the ΔarcAΔiclR strain). However, the regulatory mechanism behind this remains unclear and needs to be resolved. Compared to the wild type, the ΔarcA strain has a similar overall flux distribution which was also found by Nanchen et al. , but contradicts the data obtained by Nizam et al. 
Physiological comparison between E. coli K12 ΔarcAΔiclR and E. coliBL21
As explained in the previous sections the double knockout strain E. coli K12 ΔarcAΔiclR shows an improved formation of biomass under both glucose abundant and limiting conditions (see Figure 1), with the most distinct effect under glucose abundant conditions (50% increase). This is mainly attributed to a reduced acetate and CO2 formation. After investigation of the intracellular fluxes (Figure 5A), the higher biomass yield under batch conditions can be explained by the activity of the glyoxylate pathway and the concomitant lower CO2 loss in the TCA. Furthermore, as a result of arcA deletion, repression on TCA cycle genes is removed, resulting in a higher TCA flux and a lower acetate formation. Also a slight increase in glycogen content was noticed in this strain under both growth conditions as shown in Table 3.
Comparison of the codon usage in the arcA gene between E. coli K12 MG1655 and BL21 (DE3) based on Chen & Texada, .
Under glucose abundant conditions the double knockout strain E. coli MG1655 ΔarcAΔiclR exhibits an increased biomass yield of 0.63 c-mole/c-mole glucose, which approximates the maximum theoretical yield of 0.65 c-mole/c-mole glucose. Also under glucose limitation a higher biomass yield was observed, but effects were less distinct due to a fixed growth rate and a higher maintenance. The higher biomass formation is accompanied by a decrease in acetate formation and CO2 production. Only a small part of the higher yield was attributed to an increased glycogen content. Furthermore, enzyme activity measurements showed an increased transcription of glyoxylate enzymes, implying the activation of this pathway in the ΔarcAΔiclR strain even under glucose abundant conditions, when Crp-activation is absent. This was confirmed by 13C metabolic flux analysis, showing that 30% of isocitrate molecules were channeled through the glyoxylate pathway when iclR was knocked out. Deletion of arcA results in loss of repression on transcription of TCA genes, which provokes a higher flux through the TCA cycle. This explains the lower acetate formation observed. Because many physiological and metabolic properties observed in the double knockout strains are also attributed to E. coli BL21, the metabolic fluxes of the two strains were compared under glucose abundant conditions. Almost all fluxes in central metabolism seemed to be similar, which can be explained by mutations in the promoter region of iclR and a less efficient codon usage of arcA in BL21, resulting in lower activity of the corresponding enzymes.
List of strains used.
Coli Genetic Stock Center
ArcA knockout strain
IclR knockout strain
ArcA-IclR double knockout strain
Coli Genetic Stock Center
Luria Broth (LB) medium consisted of 10 g.L -1 tryptone peptone (Difco, Belgium), 5 g.L -1 yeast extract (Difco) and 10 g.L -1 sodium chloride. Shake flask medium (S) contained 2 g.L -1 NH4Cl, 5 g.L -1 (NH4)2SO4, 2.993 g.L -1 KH2PO4, 7.315 g.L -1 K2HPO4, 8.372 g. L -1 MOPS, 0.5 g. L -1 NaCl, 0.5 g.L -1 MgSO4 · 7 H2O, 16.5 g.L -1 glucose · H2O, 1 mL.L -1 trace element solution and 100 μL.L -1 molybdate solution. The medium was set to a pH of 7 with 1 M KH2PO4.
The minimal medium during fermentations (M1) in a benchtop bioreactor contained 6.75 g.L-1 NH4Cl, 1.25 g.L -1 (NH4)2SO4, 1.15 g.L -1 KH2PO4, 0.5 g.L -1 NaCl, 0.5 g.L -1 MgSO4 · 7 H2O, 16.5 g.L -1 glucose · H2O, 1 mL.L -1 trace element solution and 100 μL.L -1 molybdate solution.
In 13C-flux analysis experiments, minimal medium for minireactors (M2) was used. This medium contained 1 g.L -1 NH4Cl, 1 g.L -1 (NH4)2SO4, 3 g.L -1 KH2PO4, 7.315 g.L -1 Na2HPO4, 0.5 g.L -1 NaCl, 0.5 g.L -1 MgSO4 · 7 H2O, 3 g.L -1 glucose, 1 mL.L -1 trace element solution, 100 μL.L -1 molybdate solution. The glucose used in this M2 medium was added as a mixture of 20% U-13C glucose (99% purity) and 80% naturally labeled glucose or as a mixture of 50% 1-13C glucose (99% purity) and 50% naturally labeled glucose depending on the flux ratios that needed to be identified. Trace element solution consisted of 3.6 g.L -1 FeCl2 · 4 H2O, 5 g.L -1 CaCl2 · 2 H2O, 1.3 g.L -1 MnCl2 · 2 H2O, 0.38 g.L -1 CuCl2 · 2 H2O, 0.5 g.L -1 CoCl2 · 6 H2O, 0.94 g.L -1 ZnCl2, 0.0311 g.L -1 H3BO4, 0.4 g.L -1 Na2EDTA · 2 H2O, 42 g.L -1SeO2 and 1.01 g.L -1 thiamine · HCl. The molybdate solution contained 0.967 g.L -1 Na2MoO4 · 2 H2O. If not specifically mentioned, all chemicals were purchased at Sigma, Belgium.
To determine substrate uptake and product secretion rates, enzyme activities, and glycogen and trehalose contents, cells were cultivated in 2L benchtop bioreactors, since higher volume vessels improve accuracy of the measurements. However, in order to map the metabolic fluxes in the cell, expensive 13C-labeled substrates are necessary and therefore alternative miniscale reactors were chosen as the method of cultivation. Earlier studies have shown that similar growth conditions were achieved in the benchtop and miniscale reactor setups [69, 70].
For experiments in bioreactors, a preculture in a test tube filled with 5 mL LB medium was inoculated with a single colony from a LB-plate and incubated during 8 hours at 37°C on an orbital shaker at 200 rpm. From this culture, 2 mL was transferred to 100 mL minimal medium (S) in a 500 mL shake flask and incubated for 16 hours at 37°C on an orbital shaker at 200 rpm. A 4% inoculum was used in a 2L Biostat B Plus culture vessel with 1.5 L working volume (Sartorius Stedim Biotech, Germany). The culture conditions were: 37°C, stirring at 800 rpm, and a gas flow rate of 1.5 L.min -1. The pH was maintained at 7 with 0.5 M H2SO4 and 4 M KOH. The exhaust gas was cooled down to 4°C by an exhaust cooler (Frigomix 1000, Sartorius Stedim Biotech, Germany). A 10% solution of silicone antifoaming agent (BDH 331512K, VWR Int Ltd., England) was added when foaming increased during the fermentation (approximately 10 μL). The off-gas was measured with an EL3020 off-gas analyser (ABB Automation GmbH, Germany). All data were logged with the Sartorius MFCS/win v3.0 system (Sartorius Stedim Biotech, Germany). All strains were cultivated at least twice and the given standard deviations on yields and rates are based on at least 10 data points taken during the repeated experiments.
For labeling experiments miniscale reactorsetups had to be used due to the high cost of the labeled substrate. Batch conditions were achieved in 24 deepwell microtiterplates , while continuous conditions were gained by using a bubblecolumn reactor . In both cases an exponentially growing shake flask culture was used to inoculate minimal medium M2 to achieve an initial optical density (OD595 nm) of 0.02 in each well of the microtiterplate or each bubblecolumn reactor by varying the inoculation volume. 24 square deepwell plates (Enzyscreen, The Netherlands) were filled with 3 mL of M2 medium and were incubated at 37°C on an orbital shaker at 250 rpm (shaking diameter = 5 cm). Plates were closed with so called sandwich covers (Enzyscreen, The Netherlands) to prevent cross-contamination and evaporation. To further reduce evaporation, a shake flask filled with water was placed in the incubator. All strains were cultivated in at least twelvefold and in at least two different plates. The setup of the bubblecolumn reactor is described in more detail elsewhere . The working volume was 10 mL. After the batch phase was completed, a dilution rate of 0.1 h -1 was established.
In batch cultivations, samples were taken during the exponential growth phase. In continuous experiments, samples were taken after at least 7 dilution times. The sampling method was the same as earlier described . Glucose abundant conditions imply a glucose concentration higher than 5 g.L -1 in the benchtop reactor experiments (15 g.L -1 glucose in M1 medium) or higher than 1.5 g.L -1 in the miniscale reactor setup experiments (3 g.L -1 glucose in M2 medium). In batch experiments, glucose concentrations were never lower than 1 g.L -1 in the samples used for comparative analysis. This concentration is more than 15 times higher than the glucose concentration of 54 mg.L -1 at which an effect on cAMP levels (a marker of glucose limitation) can be noticed . Glucose limiting conditions imply a glucose concentration lower than 5 mg.L -1 . Samples for enzyme activity measurements or metabolic flux analysis were always taken during the mid-exponential growth phase when the glucose concentration was not limiting growth.
Determination of biomass, organic acids and glucose concentrations
The biomass content was obtained by centrifugation and subsequent drying of 20 mL reactor broth. The concentrations of glucose and organic acids were determined on a Varian Prostar HPLC system (Varian, Belgium), using an Aminex HPX-87H column (Bio-Rad, Belgium) heated at 65°C, equipped with a 1 cm reversed phase precolumn, using 5 mM H2SO4 (0.6 mL.min -1) as mobile phase. Detection and identification were performed by a dual-wave UV-VIS (210 nm and 265 nm) detector (Varian Prostar 325) and a differential refractive index detector (Merck LaChrom L-7490, Merck, Belgium). Metabolites detectable by HPLC were acetate, acetaldehyde, acetoin, ethanol, formate, fumarate, oxaloacetate, lactate, pyruvate, succinate and glucose. Product yields and (specific) product secretion rates were calculated based on end sample concentrations and maximum growth rate for MTPs and on concentrations of ten samples taken at different time points for benchtop bioreactors .
Glycogen and trehalose content
Glycogen and trehalose assays were based on the method described by Parrou et al. . In short, isoamylase, amyloglucosidase and trehalase (Sigma, Belgium) were used to degrade glycogen and trehalose to glucose. The glucose that is formed in these reactions was measured with a glucose oxidase peroxidase assay (GOD-POD). Standards were used to determine the glycogen and trehalose recovery (measured as 91% and 86%, respectively). Matrix effects were excluded by applying standard addition.
Enzyme activity assays for malate synthase and isocitrate lyase
Samples for these measurements were kept at 80°C until analysis. A predetermined amount of cells was lyzed with the EasyLyse™ cell lysis kit (Epicentre Biotechnologies, The Netherlands) and the cell extract was kept at 4°C Isocitrate lyase assay was adopted from . This colorimetric method is based on the reaction of glyoxylate, a product of isocitrate lyase, with phenylhydrazine. The reaction mixture is composed of 6 mM magnesium chloride, 4 mM phenylhydrazine, 12 mM L-cystein, and 8 mM trisodium isocitrate in a 100 mM potassium phosphate buffer (pH 7). 985 L of this mixture was added to 15 μL of enzyme extract. Enzyme activity was measured at 324 nm at 30°C (Uvikom 922 spectrophotometer, BRS, Belgium). The malate synthase assay was also adopted from . This is a colorimetric assay based on the reaction of coenzyme CoA with DTNB (5,5'-dithio-bis-(2-nitrobenzoate)). The reaction mixture of this assay is composed of 15 mM magnesium chloride, 0.2 mM acetyl-CoA, 10 mM glyoxylate and 0.2 mM DTNB in a 100 mM Tris buffer (pH 8). 900 μL of this mixture was added to 100 μL enzyme extract. The enzyme activity was measured at 412 nm at 30°C. The activity was normalized to the amount of biomass used for the assay and is expressed in μmol per minute per gram biomass.
GC-MS analysis of amino acids
The analysis of the isotopic labeling of amino acids was based on . Briefly, cell pellets, sampled at steady state (OD595 = ±1) were hydrolyzed with 6M HCl at 105°C for 24 h in sealed eppendorf tubes. Subsequently the hydrolyzates were dried in a Thermomixer (Eppendorf, VWR, Belgium) at 90°C for no longer than 12 h. Amino acids were extracted from the hydrolyzed pellet using 30 μL dimethylformamide (Acros Organics, Belgium) and derivatized with 30 μL
N-(tert-butyldimethylsilyl)-N-methyltrifluoroacetamide (MTBSTFA) + 1% tert-butyldimethylchlorosilane (TBDMSCl) (Sigma, Belgium) for 1 h at 85°C. 1 μL of this mixture was injected into a TRACE gas chromatograph connected to a DSQ mass spectrometer (Thermo, Interscience, Belgium) equipped with a TR-1 (30 m × 0.25 mm × 0.25 μm, Thermo) column. The carrier gas was helium and the flow was set at 1.5 ml.min -1 with flow mode in split control (split ratio 10.1). The oven temperature was initially kept at 160°C for 1 min and then the temperature was gradually increased to 310°C at a rate of 20°C.min -1 The final temperature was kept for 0.5 min. The injector and the ion source temperature were set at 230°C. Electron impact ionization was performed at 70eV . Mass spectra were analyzed in full scan mode from 180 to 550 amu's with a scan rate of 1400 amu.s-1. The obtained mass distribution vectors of the fragments of the amino acids were corrected for naturally occurring isotopes .
13C-Constrained metabolic flux analysis
where f1, f2 and (1 - f1 - f2) resemble the fractions of OAA molecules originating from anaplerosis, the glyoxylate shunt, and the TCA cycle, respectively. The labeling of a molecule X in this equations is expressed as Xa-bwhere a-bindicates the carbon atoms considered. C1 is a one carbon atom with the fractional labeling of the input substrate.
To solve this equation, a Monte-Carlo approach was implemented in Matlab. First, average mass distribution vectors (mdv's) and standard deviations for every Xa-bwere calculated based upon at least 10 GC-MS analyses of different biological samples. Next, samples were taken in the mdv measurement matrix using the normrnd function. Finally, the equation was solved by varying f1, f2 and the fractional labeling of CO2 and the best fit solution was kept. Step 2 and 3 of this calculation process were repeated 1000 times and all values of f1, f2, and the measured labeling of CO2 were plotted to check if the parameters were normally distributed. If this was valid, average values and standard deviations for these parameters were calculated.
Subsequently, intracellular fluxes were calculated in the NETTO module of Fiatflux, using a slightly modified version of a previously described stoichiometric model , extended with succinate transport out of the cell. This model consisted in total of 27 reactions and 22 balanced metabolites. Glucose uptake, succinate and acetate excretion were experimentally determined. The effluxes of precursor metabolites to biomass formation was estimated based on the growth rate dependent biomass composition of E. coli [80–82]. The underdetermined system of equations with 5 degrees of freedom was solved by using the following 7 ratios as constraints: Serine from glycolysis, Pyruvate through ED pathway, Pyruvate from malate (upper and lower bound), OAA originating from PEP, OAA originating from glyoxylate, and PEP originating from OAA.
This work was financially supported by the Special Research Fund (BOF) of Ghent University and performed in the framework of the SBO project MEMORE 040125 of the IWT Flanders. The authors like to thank Nicola Zamboni and Stephen Busby for lively scientific discussions.
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