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Overflow metabolism in the presence of oxygen occurs at fast growth rates in a wide range of organisms including bacteria, yeast and cancer cells and plays an important role in biotechnology during production of proteins or metabolic compounds. As recently suggested, overflow metabolism can be understood in terms of proteome allocation, since fermentation has lower proteome cost for energy production than respiration. Here, we demonstrate that ArcA overexpression in aerobic conditions, results in downregulation of respiratory pathways and enhanced growth rates on glycolytic substrates of E. coli, coinciding with acetate excretion and increased carbon uptake rates. These results suggest that fermentation enables faster growth and demonstrate that fermentation on many glycolytic carbon sources is not limited by carbon uptake. Hence, these findings are difficult to reconcile with many alternative hypotheses that have been proposed for the origin of overflow metabolism and the growth rate dependence of fermentation and respiration, which are based on limited capacity of respiration or limitations in uptake rates and catabolic pathways. Instead, as suggested by increased lag phases of ArcA overexpression strains, respiratory energy metabolism may be related to a general preparatory response, observed for decreasing growth rates, but with limited advantages for maximizing steady-state growth rate.
Respiration and fermentation are alternative metabolic strategies for energy production. To supply energy required for their survival and growth, many organisms, including E. coli, use different combinations of respiration and fermentation depending on their environments and growth conditions1–3. Fermentation involves the excretion of byproducts such as acetate or lactate4, whereas using respiration, carbon is fully oxidized to CO2. As a consequence, a much lower amount of ATP per molecule of metabolized substrate is produced from fermentation compared to respiration. Nevertheless, fast-growing microbial cells, ranging from E. coli 5 and yeast6, and fast-growing mammalian cells like tumor cells or stem cells7,8, heavily rely on fermentation for their energy requirements, even in the presence of oxygen.
In previous work3, we demonstrated that the patterns of acetate excretion in E. coli under different growth limitations can be explained by a proteome allocation model. The metabolic advantage of fermentation over respiration is due to a lower investment in the protein machinery required to produce the necessary ATP flux for rapid growth. Hence, fermentation constitutes a “leaner” pathway, where abundant carbon can be “wasted” by excretion. Our previous study quantitatively explains interrelations between growth rates, carbon uptake rates, acetate excretion rates, as well as patterns of gene expression that are observed under diverse conditions. However, important questions regarding the underlying rationale of these patterns remain, in particular, the reason for the heavy reliance on respiration observed for many glycolytic carbon sources3,9, when fermentation should be advantageous for fast growth. It is unclear why E. coli strains grow slowly on many glycolytic substrates, and use respiration exclusively to meet their energy needs, even when the carbon source is highly abundant in the medium. Even at faster growth rates, it is unclear why bacteria use a combination of fermentation and respiration3, instead of concentrating all their resources on the “leaner” pathway. The proteome cost of most carbon specific operons is comparatively small10 and therefore, from the perspective of growth rate maximization, cells should be able to increase their uptake rates to take advantage of fermentation for energy production. Have E. coli strains simply not learned to express higher levels of carbon transporters on these substrates, or are there fundamental limitations to carbon uptake rates? Or do these slow growth rates arise from as yet unappreciated objectives other than growth rate maximization?
Here, to elucidate these questions, we directly tested the effect of repressing respiration on growth rates of E. coli. We demonstrate that forcing E. coli K12 strains to increase fermentation of glycolytic carbon sources results in enhanced growth rates, lower biomass yield and higher carbon uptake rates. Reflecting a lower protein cost fermentation, these results buttress our previous findings3, but challenge the commonly held notion that the heavy reliance on respiration for metabolism of many glycolytic carbon sources is caused by fundamental limitations in carbon availability or uptake.
A genetic construct was engineered that allowed repression of respiration in E. coli, by controlled overexpression of the global transcriptional regulator ArcA, using the linearly titrable Ptet/tetR system11 (see Fig. S1). Normally, under anaerobic conditions, ArcA is phosphorylated by its membrane counterpart ArcB, and ArcAP represses genes involved in respiration such as enzymes in the TCA cycle12. Here, we show that overexpression of ArcA results in downregulation of aerobic metabolic pathways even under aerobic conditions, forcing cells to rely more on fermentation for energy production.
Using this overexpression system, the growth physiology for different ArcA induction levels on minimal medium was characterized with various carbon sources, revealing a remarkable effect. While high ArcA expression levels were detrimental for growth, presumably by repressing the TCA cycle below levels required for the production of biomass precursors, intermediate ArcA levels resulted in significantly faster growth on many glycolytic carbon sources, as shown for fructose and mannose in Fig. 1a (control strain, Fig. S2a). Testing a range of glycolytic carbon sources with varying growth rates, improved growth rates were observed at intermediate ArcA overexpression levels for all carbons tested (Fig. 1b). Glycolytic carbons that allow fast growth rates of wildtype E. coli like glucose and lactose only exhibited a small, but reproducible improvement of their growth rates. But “slow” glycolytic carbon sources like mannose, on which wildtype E. coli exclusively utilizes respiratory pathways1,10, showed substantial growth rate improvements with intermediate ArcA overexpression. This improved growth rate of ArcA overexpression strains on glycolytic carbons was in marked contrast to the effect of ArcA for growth on TCA carbons such as succinate, where even moderate overexpression of ArcA had a strongly detrimental effect on growth rates (see Fig. S2b). The relative growth rate improvement as a function of the growth rate without ArcA overexpression is shown for different glycolytic carbon sources in Fig. 1b.
Improved growth rates suggest that ArcA overexpression results in the substitution of fermentation for respiration. To confirm this, the excretion rate of acetate, the main fermentation product of E. coli, was measured for different ArcA overexpression levels. Indeed, ArcA overexpression led to increased acetate excretion (Figs 2a and S3). In particular, acetate excretion appeared with poor carbon substrates such as mannose, where acetate production is absent in the wildtype3 and without ArcA induction.
The increase in growth rate and the excretion of fermentation products should coincide with a decrease in biomass yield and an increased carbon uptake rate. The saturating optical density (OD600) with low initial concentrations of different carbon sources was measured and for different levels of ArcA overexpression. As anticipated, cultures with ArcA overexpression ran out of carbon and stopped growing at lower culture densities (see Fig. S4). Together with the higher growth rates that we observe, this means that ArcA overexpression strains have higher carbon uptake rates. We note that acetate levels in these experiments are far below growth inhibitory concentrations.
To test if the growth rate enhancing effect of ArcA overexpression was specific to the NCM3722 strain13, the ArcA overexpression construct was introduced into the BW25113 background14. The enhanced growth rates and increased acetate excretion were also observed in this background (Fig. S5).
In order to directly study the effect of ArcA overexpression on gene expression, a set of β-galactosidase reporter constructs was engineered for genes involved in respiratory pathways. Expression levels measured this way are plotted against induction levels of ArcA overexpression in Fig. 2b. Indeed, ArcA overexpression was effective at repressing respiratory genes, affecting TCA genes more strongly than the glyoxylate shunt. Maximum growth rates were achieved for intermediate levels of respiratory genes. On the other hand, strong downregulation of respiratory genes often had a detrimental effect on growth rate, presumably because these pathways are required for the production of biomass precursors, as quantified in our previous work3. To gain a genome scale picture of the changes in gene expression resulting from ArcA overexpression, we employed quantitative proteomic mass spectrometry to track the relative changes in abundance of a large number of proteins (Fig. 2c). Consistent with the results from reporter constructs, proteomics revealed the global downregulation of respiratory pathways with ArcA overexpression. It is likely that the repression of non-essential proteins outside respiratory metabolism also contributes to the enhanced growth rates under ArcA overexpression (Fig. 2d).
Several other genetic alterations are known to lead to faster than wildtype growth rates on one or several carbons. These mutations include the knockout of flagellar genes (ΔflhD)3, growth on glycerol with mutations of an allosteric fructose 1,6-bisphosphate binding site in glycerol kinase GlpK15, as well as recent findings on the optimal level of cAMP16. The knockout of the global transcriptional regulator of glycolysis and gluconeogenesis cra exhibits similarly striking improvements in growth rate for a number of glycolytic carbon sources. Δcra strains cannot grow on many gluconeogenic carbon sources, as transcriptional activity of cra represses glycolytic enzymes and activates gluconeogenesis17,18. Therefore, we suspected that the high growth rate, fermentative phenotype of ArcA overexpression could be enhanced by the cra knockout. The ArcA overexpression system was introduced into a Δcra-background, and growth on mannose minimal medium was tested. Indeed, the effects of Δcra and ArcA overexpression were additive, with a resulting growth rate that was roughly twice as fast as the growth rate of the wildtype strain on mannose minimal medium (Fig. S7).
Our results demonstrate that downregulation of respiratory pathways via controlled overexpression of the global regulator ArcA in E. coli, remarkably leads to faster growth rates on a large number of glycolytic carbon sources. The largest increase in growth rate was observed for ‘slow’ glycolytic carbon sources such as mannose, on which wildtype E. coli normally exclusively relies on respiration for energy production. Acetate excretion could be induced even on these ‘slow’ carbon sources and hence, the threshold growth rate for acetate excretion was decreased by ArcA overexpression3. The increase in growth rates with ArcA overexpression coincided with increased acetate excretion, a decreased biomass yield and increased carbon uptake rates. The downregulation of genes involved in respiration by ArcA overexpression was verified using reporters of gene expression, as well as proteomics.
We note that it may be possible to increase growth rates even more, because ArcA overexpression likely does not result in perfect substitution of respiration by fermentation, including sufficiently high uptake rates, required for perfect compensation of the loss of respiraton. ArcA overexpression may also have regulatory effects beyond energy metabolism. However, our results demonstrate that the upregulation of respiration pathways on “slow” glycolytic carbons is not caused by limitations of carbon uptake, as commonly believed, because significantly faster growth rates fueled by even higher uptake rates are evidently possible. Instead, we argue that the observed utilization of respiratory pathways like the TCA and glyoxylate cycle on slow glycolytic carbon sources1, as well as other recent findings regarding suboptimal growth rates16, arise from different objectives, other than maximizing steady-state growth rate, and may be part of a global preparatory response for adaptation to changing environments. As one example, in a study in preparation, we show a direct dependence of lag times resulting from carbon shifts on growth rates and glycolytic flux, with fast growth rates resulting in very long lag phases, consistent with previous findings19 and with growth rate improvements of the cra knockout (Fig. S7). Indeed, ArcA overexpression before carbon shifts resulted in substantially increased lag times (Fig. S8).
Finally, we note that ArcA overexpression or ArcB activation12,20, which shows even stronger repression of respiration, should be a useful tool for biotechnology applications, like for the production of metabolites. At high levels, ArcA/ArcB activity fully represses unwanted biomass production and virtually stops growth, while resulting in a large fermentative metabolic flux that could be diverted to desired products. This is similar to the effect of anaerobic conditions, a common strategy for maximizing production yield, but ArcAB activation can result in a stronger inhibition of biomass production and has the added advantage of allowing efficient energy metabolism via the electron transport chain.
The arcA gene including the 5’-UTR was amplified from genomic DNA of NCM3722 using primers Ptet-ArcA-XhoI-F and ArcA-BamHI-R. The Ptet promoter sequence, as well as an XhoI site were included in the forward primer Ptet-ArcA-XhoI-F. A BamHI site was included in the reverse primer ArcA-BamHI-R. The resulting DNA fragment was used to replace Ptet-gfp in the plasmid pZA31-gfp(Levine et al., 2007) yielding the plasmid pZA31 Ptet-arcA. This plasmid was then transformed to various backgrounds. The plasmid pZA31 Ptet-RF was characterized in a previous study(Levine et al., 2007).
The aceB promoter region (−191 bp to +204bp relative to the aceB translational start point), the fumA promoter region (−426 bp to +216bp relative to the fumA translational start point), the sdhC promoter region (−231 bp to +380bp relative to the sdhC translational start point) and the lpd promoter region (−222 bp to +359bp relative to the lpd translational start point) were amplified from genomic DNA of NCM3722. These DNA fragments were then inserted between the XhoI and BamHI sites downstream of the rrnB terminator (rrnBT) in pKDT(Klumpp et al., 2009), yielding the plasmids pKDT-PaceB, pKDT-PfumA and pKDTPsdhC, respectively. Using each of these plasmids as template, the DNA region containing the km r gene, rrnBT and the promoter was PCR amplified and subsequently integrated into the chromosome of E. coli strain NQ309 to replace part of lacI and the entire PlacZ (from +134bp after the lacI translational start codon to the lacZ translational start codon)(Datsenko & Wanner, 2000). Then each of the promoter-lacZ fusions was transferred to different genetic backgrounds by phage P1 vir mediated transduction.
The Δcra deletion allele in strain LJ2801 (E. coli Genetic Stock Center, Yale Univ.), in which a km r gene is substituted for the cra gene, was transferred to wildtype NCM3722, resulting in the strain NQ1077.
NC- minimal medium (Csonka et al., 1994), which contains K2SO4 (1g), K2HPO4.3H2O (17.7g), KH2PO4 (4.7g), MgSO4.7H2O (0.1g), and NaCl (2.5g) in one liter, and is supplemented with various carbon and nitrogen sources. For carbon limited growth of wild-type cells, 20mM NH4Cl were used. For carbon sources concentrations were based on the number of carbon atoms in the molecule: 20mM for C6-carbons, 30mM for C4-carbons and 40mM for C3-carbons.
Batch culture growth was performed in a 37°C water bath shaker shaking at 250rpm. The culture volume was at most 10ml in 25 mm × 150 mm test tubes. Each growth experiment was carried out in three steps: seed culture in LB broth, pre-culture and experimental culture in identical minimal medium. For seed culture, one colony from fresh LB agar plate was inoculated into liquid LB and cultured at 37°C with shaking. Cells were then diluted into the minimal medium and cultured in 37°C water bath shaker overnight (pre-culture). The overnight pre-culture was allowed to grow for at least 3 doublings. Cells from the overnight pre-culture was then diluted to OD600=0.005–0.025 in identical pre-warmed minimal medium, and cultured in 37°C water bath shaker (experimental culture). 200 μl cell culture was collected in a Sterna Sub-Micro Cuvette for OD600 measurement using a Thermal Spectrophotometer every half doubling of growth. The time taken for each sample collection is <30sec and had no measureable effect on cell growth.
The assay was performed following a similar protocol as detailed in a previous study6. 100μL samples were taken for at least 4 different times during exponential growth (typically at OD600 between 0.1 and 0.6). LacZ samples were immediately added to 0.9mL of freshly prepared Z-buffer (in 1L: 8.52g Na2HPO4, 5.5g NaH2PO4•H2O, 0.75g KCl and 0.25g MgSO4•7H2O, with 0.004%(w/v) SDS and 40mM β-mercaptoethanol) with 100μL chlorophorm. Cells were disrupted by vortexing and stored at 4°C until all samples were collected. After all samples were collected, they were briefly vortexed a second time. After 5–10minutes at room temperature to settle the chlorophorm, the lysates were diluted (typically 1:4) in Z-buffer. 200μL was then added to a 96-well plate (Sarstedt). Immediately prior to reading in GENiosPro (Tecan) plate reader, 40μL of of 4mg/mL Ortho-Nitrophenyl-β-galactoside (Sigma) in 0.1M phosphate buffer (pH=7.0) was added to each well. The plate reader was set to read absorbance at a wavelength of 420nm every minute for 60 to 120minutes at 28°C.
The slope of the plot of OD420 vs. time (in minutes) for all replicates was used to calculate the β-galactosidase activity (Units/mL) in the original sample via the following conversion:
where the fold dilution is from both the initial dilution of cell sample in Z-buffer/chloroform and the dilution of lysates in Z-buffer before being loaded to the plate. The factor 2.66 converts the plate-reader data to the activity obtained using the original assay protocol by Miller, and is specific to the path-length through the sample (i.e. 240μL in a 96-well plate). The slope of the plot of activity (Units/mL) versus the sample OD600 yields theactivity in Miller units (Units/mL/OD600).
200μL samples were taken and immediately frozen. Before the assay, samples were thawed in water and immediately centrifuged at maximum speed (15,000rpm) for 2.5min. 100μL of supernatant were used to measure acetate concentrations using the Acetate Assay kit (Catalog #:10148261035, R-Biopharm).
For each of the cultures, 1.8ml of cell culture at OD600=0.4~0.5 was collected by centrifugation. The cell pellet was re-suspended in 0.2ml water and fast frozen on dry ice.
Aliquot of the mixture of the two 15N labeled cell samples was mixed with each of the non-labeled cell samples, which contained the same amount of proteins (~100µg proteins). Proteins were precipitated by adding 100% (w/v) trichloroacetic acid (TCA) to 25% final concentration. Samples were let stand on ice for a minimum of 1hour. The protein precipitates were sped down by centifugation at 16,000g for 10min at 4°C. The supernatant was removed and the pellets were washed with cold acetone. The pellets were dried in a Speed-Vac concentrator. The pellets were dissolved in 80µl 100mM NH4HCO3 with 5% acetonitrile (ACN). Then 8µl of 50mM dithiothreitol (DTT) was added to reduce the disulfide bonds before the samples were incubated at 65°C for 10min. Cysteine residues were modified by the addition of 8µl of 100mM iodoacetamide (IAA) followed by incubation at 30°C for 30min in the dark. The proteolytic digestion was carried out by the addition of 8µl of 0.1µg/µl trypsin (Sigma-Aldrich, St. Louis, MO) with incubation overnight at 37°C. The peptide solutions were cleaned by using the PepClean® C-18 spin columns (Pierce, Rockford, IL). After drying in a Speed-Vac concentrator, the peptides were dissolved into 10µL sample buffer (5% ACN and 0.1% formic acid).
The peptide samples were analyzed on an Agilent G6520B TOF mass spectrometer. Peptides were eluted from a 90-min, 5–60% concave acetonitrile gradient. The precursor mass window was from 400 to 2000 m/z and the product ion mass window from 80 to 2000 m/z. Fragmentation were collected under the data-dependent Auto MS/MS mode with 1sec scan cycle times, 4 maximum precursors per cycle, a 1500 abundance threshold, and active exclusion after 2 spectra for 5min.
The raw mass spectrometry data files generated by the Agilent G6520B TOF system were converted to Mascot generic format (mgf) files, which were submitted to the Mascot database searching engine (Matrix Sciences, London, UK) against the E. coli SwissProt database to identify proteins. The following parameters were used in the Mascot searches: maximum of two missed trypsin cleavage, fixed carbamidomethyl modification, variable oxidation modification, peptide tolerance ±0.1Da, MS/MS tolerance±0.1Da, and 1+, 2+, and 3+ peptide charge. All peptides with scores less than the identity threshold (P=0.05) were discarded.
The raw mass spectrometry data files were converted to the.mzMLfiles. Results of the Mascot search were submitted with.mzML files to our in-house quantification software(Sperling et al., 2008). Briefly, intensity is collected for each peptide over a box in RT and m/z space that encloses the envelope for the light and heavy peaks. The data is collapsed in the RT dimension and the light and heavy peaks are fit to a multinomial distribution (a function of the chemical formula of each peptide) using a least squares Fourier transform convolution routine(Sperling et al., 2008), which yields the relative intensity of the light and heavy species. The ratio of the non-labeled to labeled peaks was obtained for each peptide in each sample.
The relative protein quantitation data for each protein in each sample mixture was then obtained as a ratio by taking the median of the ratios of its peptides. No ratio (i.e., no data) was obtained if there was only one peptide for the protein. The uncertainty for each ratio was defined as the two quartiles associated with the median. To filter out data with poor quality, the ratio was removed for the protein in that sample if at least one of its quartiles lied outside of 50% range of its median; Furthermore, ratios were removed for a protein in all the sample mixtures in a growth limitation if at least one of the ratios has one of its quartiles lying outside of the 100% range of the median.
Proteome fractions of cells grown on mannose minimal medium with no chlortetracycline were taken from previously quantified proteome fractions for carbon-limiting cells that have the same growth rate (NCM3722-background strain with glycerol uptake titrated)(Hui et al., 2015). The proteome fraction for a protein in cells with a given level of chlortetracycline was then calculated by multiplying the protein’s proteome fraction in the zero-chlortetracycline condition with its expression level relative to the zero-chlortetracycline condition.
To establish our central finding (error bars in Fig. 1b, main text), the increased growth rate with ArcA overexpression, growth rate curves versus inducer curves for ArcA overexpression were repeated independently multiple times for multiple carbon sources (mannose: 6 repeats; fructose: 6 repeats; glucose: 6 repeats; glycerol: 2 repeats). Error bars for saturating OD600 were established from repeats on mannose minimal medium (Fig. S4). Based on experience from previous work (Basan et al., 2015), for measurements of acetate excretion rates resulting from four acetate measurements along the growth curve, we assumed 15% relative errors.
We are grateful to Terry Hwa and Uwe Sauer for many discussions and supporting this research, as well as to the members of their labs. This work was financially supported by the NIH (R01-GM109069 and GM118850 to JRW) and the Simons Foundation (Grant 330378).
M.B., S.H. and J.R.W. designed the study. M.B. and S.H. performed the experiments. M.B., S.H. and J.R.W. wrote the paper.
The authors declare that they have no competing interests.
Electronic supplementary material
Supplementary information accompanies this paper at 10.1038/s41598-017-12144-6.
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