Enhancing the Glucose Flux of an Engineered EP-Bifido Pathway for High Poly(Hydroxybutyrate) Yield Production

Introduction

In 2018, global carbon dioxide emissions increased 1.7% over the previous year, hitting a record high of 33.143 billion tons. Accelerating the adoption of renewable energy and improving energy efficiency in response to global warming are urgent priorities (International Energy Agency, 2019). Bio-manufacturing, which uses food crops as raw materials, has wide application prospects. Through biological manufacturing, biomass resources can be converted to ethanol, polylactic acid, 1, 3-propanediol, and other bulk chemicals (Ragauskas et al., 2006; Lee et al., 2012). A key barrier to this process is the CO₂ emissions that occur during natural aerobic fermentation. Many carbon dioxide fixation pathways have been exploited using the six carbon fixation pathways discovered in nature (Gong et al., 2016). However, complex reaction steps and enzyme requirements limit the broad application of these carbon sequestration pathways (Erb et al., 2007; Schwander et al., 2016).

In natural microorganism fermentation, glucose can be transformed through the Embden-Meyerhof-Parnas (EMP) pathway to pyruvate. Pyruvate metabolism leads to the production of two molecules of acetyl-CoA (AcCoA), the key precursor of ethanol, butanol, fatty acids, amino acids, and pharmaceuticals. This process produces two molecules of CO₂ from one mol of glucose, making it an uneconomical way to biosynthesize products using AcCoA as precursor. Other glycol metabolism pathways, such as the phosphoketolase pathway, employ a pentose phosphate specific transketolase to produce a mixture of ethanol, lactic acid, and CO₂. Additionally, the bifido bacteria exclusive bifid shunt pathway can generate 1 mol of lactic acid and 1.5 mol of acetate from 1 mol of glucose (Meile et al., 2001; Posthuma et al., 2002). However, all of these glucose metabolic pathways lose carbon in the form of CO₂ during the decarboxylation process. Therefore, several carbon-saving pathways, including the non-oxidative glycolytic (NOG) and EP-bifido pathways, have been engineered. The NOG pathway can transform all six carbon atoms of glucose into three AcCoA molecules without CO₂ loss (Bogorad et al., 2013). However, it cannot provide the reducing power NADPH that is needed for PHB and other chemicals biosynthesis. The EP-bifido pathway employs EMP, pentose phosphate pathway (PPP) and the Bifido shunt for high-yield of AcCoA generation. As a reducing power sponsor, the oxidation part of the PPP consumes 1 mol of glucose, and provides 2 mol of NADPH and 1mol of xylulose-5-phosphate (X5P). The enzyme encoded by the f/xpk gene of the EP-bifido pathway has both fructose-6-phosphate (F6P) and X5P activity. It is able to catalyze X5P to form acetyl phosphate (AcP) and glyceraldehyde 3-phosphate (G3P) or split F6P to form erythrose 4-phosphate and AcP. The former G3P can generate AcP through carbon rearrangement, each of these processes releases only 1 mol of CO₂, thus saving the carbon source to a certain extent (Figure 1). This carbon-saving pathway has been applied to the production of several compounds that use AcCoA as the precursor (Wang et al., 2019). Previously, we achieved a relatively high level of production and yield, but there remains room to improve carbon conversion in our system.

FIGURE 1

Figure 1. EP-bifido pathway and theory carbon flux distribution. Metabolic optimization of EP-bifido pathway. The red box referred to the carbon rearrangement procedure. Overexpressed genes are shown in red. Deleted genes are shown in blue. Intermediate metabolites participated in carbon rearrangement are shown in orange.

In Escherichia coli, glucose is transported through the phosphate transferase system (PTS). This system is involved in phosphoenolpyruvate (PEP)-dependent sugar transport and its activity has an important impact on carbon flux redistribution in the PEP and pyruvate nodes (Gosset, 2005). Glucose was phosphorylated to G6P by the phosphoryl generated from PEP, which was dephosphorylated to form pyruvate. Then pyruvate further decarboxylated to AcCoA and released 1 mol of CO₂, leading to the loss of the carbon source. In addition, PEP is a key intermediate metabolite of the EMP pathway. Therefore, an increase in the EMP pathway reduces the carbon conversion efficiency of the EP-bifido pathway.

Poly(hydroxybutyrate) (PHB) is the most common poly(hydroxyalkanoate) (PHA). PHB can be synthesized and accumulated by more than 300 microorganisms as both an energy and carbon store (Lee and Choi, 2001; van der Walle et al., 2001). The in vivo biosynthesis of PHB requires three steps using AcCoA as the precursor, and PHB production has been intensively studied (Lee et al., 1994; Wang Q. et al., 2009). Many strategies have been applied to engineer E. coli to improve PHB production, however, the yield still has much room to progress. By overexpressing NAD kinase, recombinant E. coli produced 14 g/L PHB and the yield based on glucose reached 0.31 mol/mol (0.15 g PHB/g glucose) (Li et al., 2009). By applying fed-batch strategy, E. coli could accumulate 125 g/L PHB, but the yield based on glucose was only 0.46 mol/mol (0.22 g PHB/g glucose) (Mozumder et al., 2014). Previously, we have achieved relatively high level of PHB content and PHB yield (68.4 wt% and 63.7% mol/mol, respectively) (Wang et al., 2019). In this study, we optimized the EP-bifido pathway for improved PHB production in E. coli. The non-PTS glucose transport pathway genes glk, galP and heterogeneous glf were enhanced and introduced into EP-bifido strains through multiple automated genome engineering (MAGE) and conditional-replication, integration, excision, and retrieval (CRIM) plasmids. The improved PHB production indicates that our modification increased the efficiency of artificial carbon-saving pathways for high carbon conversion rate from glucose.

Materials and Methods

Culture Media and Conditions

For plasmid preparation, E. coli strains were cultured at 37°C on a rotary shaker (220 rpm) in test. For plasmid preparation, E. coli strains were cultured at 37°C on a rotary shaker (220 rpm) in test tubes containing 5 mL Lysogeny broth (LB) medium. For PHB biosynthesis, 50-mL shake flask cultures were started by 2% inoculation from the 5-mL LB culture. The 50-mL cultures contained M9 minimal medium with 0.2% yeast extract containing 20 g/L glucose and shaken at 37°C in a rotary shaker (120 rpm) for 48 h. Overnight cultures were shaken at 37°C in a rotary shaker (220 rpm). Antibiotics were added as follows: ampicillin (Amp) 100 μg/mL, spectinomycin (Spc) 50 μg/mL, and chloromycetin (Cm) 25 μg/mL. For MAGE procedure, strains were cultivated in SOB medium.

Lysogeny broth medium contains (g/L): tryptone (10), yeast extract (5), and NaCl (10). M9 medium contains (g/L): Na₂HPO₄⋅12H₂O (15.138), KH₂PO₄ (3), NaCl (0.5), and NH₄Cl (1). SOB medium contains (g/L): tryptone (20), yeast extract (5), and NaCl (5).

Strains and Plasmids

All E. coli strains and plasmids used are listed in Table 1. DH-EP was used as the starting strain for further genetic manipulation. All primers used for molecular manipulations are listed in Table 2.

TABLE 1

Table 1. Bacterial strains and plasmids used in this study.

TABLE 2

Table 2. Key oligonucleotide primers used in this study for DNA manipulation.

The Red homologous recombination method was employed for gene deletion. The pTKRED complementary plasmid was transformed into the target strain. Deletion fragments of ptsG gene were amplified from the JW1087-2 single-gene knockout mutant (Baba et al., 2006) (bought from Coli Genetic Stock Center, CGSC) using primers Q-ptsG-F/Q-ptsG-R.

Measurement of Extracellular Metabolites

A spectrophotometer was used to measure the optical density at 600 nm (OD₆₀₀) of the bacterial culture. PHB was quantified using gas chromatography (GC). Cells were harvested by centrifugation at 6,000 × g for 10 min, 4°C. The cell pellets were washed twice with distilled water and lyophilized for 7 h. Before GC analysis, 1 mL chloroform, 850 μL methanol, and 150 μL sulfuric acid (98%, w/w) were added to the weighed cells in vials. The vials were incubated at 100°C for 1 h. Then, 1 mL water was added for stratification and cooling vials. After standing for 1 h, the mixture separated into layers and the heavier chloroform phase was transferred to new vial for GC analysis. The GC detection process was performed using a Shimadzu GC2010 gas chromatograph (Kyoto, Japan) equipped with an AOC-20i auto injector and a Restek Rtx-5 column. PHB standard samples of methyl-(R)-3-hydroxybutyrate (Sigma-Aldrich) were dissolved in chloroform and analyzed by GC. The temperature program used was: 80°C for 1 min, ramped to 120°C at 10°C/min, then ramped to 160°C at 45°C/min for 5 min, and the total time was 10.89 min.

For extracellular metabolite analysis, 1 mL of culture was centrifuged at12,000 × g for 2 min. The supernatant was filtered through a 0.22-μm syringe filter for high-performance liquid chromatography analysis. Glucose, acetate, and pyruvate were measured on an ion exchange column (HPX-87H; Bio-Rad Labs) with a differential refractive index detector (Shimadzu RID-10A). A 0.5-mL/min mobile phase using a 5-mM H₂SO₄ solution was applied to the column. The column was operated at 65°C.

MAGE Procedure

The ribosome binding sites (RBSs) designed for the modulation of GalP and glk transcription rates were 5′-GTCGTACTC ACCTATCTTAATTCACAATAAAAAATAACCADDRRRRRD DDDATCATGCCTGACGCTAAAAAACAGGGGCGGTCAAA CAAG-3′ (D = A, G, T; and R = A, G) and 5′-GCCGCCCACA TCACCGACTAATGCATACTTTGTCATTCTHHHHYYYYYH HGCTAAAGTCAAAATAATTCTTTCTCACACTGTAAATAC CT-3′ (H = T, C, A; and Y = T, C), respectively, with four phosphorothioated bases at the 5′ terminus. The initiation of MAGE requires that pTKRED was transformed into the target strain. The MAGE cycles were performed by growing DH-EPP in 5 mL SOB medium at 30°C and shaking at 220 rpm for 12 h. For the first MAGE round, 5-mL shake flask cultures using SOB broth were started with a 1% inoculation from the overnight culture. Isopropyl-β-D-thiogalactopyranoside (IPTG) was added to a final concentration of 0.5 mM to induce λ-prophage (bet, gam, and exo) gene expression. Cells were then incubated at 30°C and shaking at 220 rpm until reaching an OD₆₀₀ of 0.5 to 0.6. Cells were collected (2 mL), pelleted, and washed three times with cold sterile water to make them electrocompetent. ssDNA mixture (1 μM) was added to electrocompetent cells and electroporated at 2.5 kV. To start the second MAGE round, cells were recovered in 5 mL SOC with IPTG until their OD₆₀₀ reached 0.5 to 0.6, after which cells underwent pelleting, washing, and electroporation. Three to four MAGE rounds were performed per day and 16 cycles were performed in total. The resulting pool of variants were then characterized using the Nile red assay.

Screening of PHB Competent Cells by Nile Red Assay

When PHB is combined with Nile red dye a red color is produced. We transformed the pCAB plasmid into these variants and added 100 μL Amp, 50 μL IPTG, 20 g/L glucose, and 200 μL Nile red dye to the solid M9 medium supplemented with 0.2% yeast extract. The MAGE variants were diluted 200-fold and spread onto several plates. After incubation at 37°C for 16 h, the plates were placed at 4°C for 3 days to allow the color reaction to develop. Based on the color difference, we picked single red colonies for sequencing. For all the sequenced colonies with mutations identified, the pTKRED plasmid was removed and the strains were transformed with the pFF and pCAB plasmids for further verification of the PHB competent cells.

Integration of glf

For glf integration, the trc-rbs-glf module was amplified from Zymomonas mobilis genomic DNA by PCR using primers GLF-F and GLF-R. The PCR product (trc-rbs-glf) was cloned into a vector that carries R6K replicon and phage attachment sites (attP). This plasmid was named R6K-glf and was confirmed by DNA sequencing. The pAH69 helper plasmid was transformed into the L-6 strain. The target strain carrying pAH69 was incubated overnight at 30°C and transferred to 37°C for 1 h before transfection. Then the pR6K-glf plasmid was introduced into L-6 by electroporation. The centrifuged bacteria were plated onto plates containing 25 μg/mL kanamycin for overnight incubation at 37°C. R6K-glf positive transformants were selected by their kan^R phenotype and were verified by PCR.

Determination of CO₂ Emissions

CO₂ emission was determined using a thermostatic oscillation incubator with a CO₂ detector (BCP-CO₂, Bluesens, Germany) that monitored CO₂ volume every 20 s and transmitted the data to a computer. Cultures were grown at 37°C with shaking at 150 rpm.

Results

Inhibiting PTS to Reduce PEP Consumption

In E. coli, glucose is transported through the PTS system. This system is involved in PEP-dependent sugar transport and its activity has an important impact on carbon flux redistribution in the PEP and pyruvate nodes (Gosset, 2005). Glucose transport into the cytoplasm by EIICB^Glc (encoded by ptsG) is coupled to its phosphorylation. The phosphate group is derived from PEP and is transferred via a cascade of proteins, enzyme I (EI), HPr, EIIA, and EIIB. This procedure consumes almost half of the PEP (Valle et al., 1996; Wang et al., 2012). Glucose was phosphorylated to G6P by phosphoryl generated from PEP dephosphorylated to pyruvate, the formed pyruvate is further decarboxylated to AcCoA and releases 1 mol CO₂, leading to carbon source loss. While PEP is not the precursor in our study, PEP consumption would convert carbon flux to the EMP pathway, which is not desirable in our EP-bifido pathway. Therefore, modulation of the PEP-independent uptake and phosphorylation system is required. Knocking out ptsG and replacing it with other glucose transport pathways is a common method used in the production of PEP-precursor products (Gosset, 2005; Lee et al., 2005; Li et al., 2013; Kyselova et al., 2018). Therefore, we knocked out ptsG in strain DH-EP and named the strain DH-EPP. But found that ptsG deletion severely impaired the growth capacity of the resulting strain. Compared with DH-EP (pFFpCAB) strain, PHB yield of DH-EPP strain decreased from 63.7 to 26.3% (mol/mol) (Figure 2).

FIGURE 2

Figure 2. Fermentation result of ptsG knockout strain. The date of PHB yield and content of both strains were calculated based on fermentation samples at 60 h. The time axis at the top was used to depict growth curve. The growth carve was showed in orange red. The experiments were performed in duplicate and error bars indicate s.d. Strains were cultivated with M9 at 37°C, 150 rpm.

For glucose uptake recovery, replacing PTS with an alternative PEP-independent uptake and phosphorylation system could be an efficient solution to this problem.

Improving Glucose Flux Through Non-PTS Pathway

When E. coli strains lack PTS, the low affinity galactose: H⁺ symporter, GalP, encoded by galP, is induced. Glucose internalized by GalP must be phosphorylated by glucokinase (encoded by glk), which catalyzes the ATP-dependent phosphorylation of glucose to generate G6P in the cytoplasm without CO₂ emission, thus saving the carbon source (Gosset, 2005). Therefore, we modified galP and glk expression levels to improve the glucose utilization rate. While increasing galP and glk transcriptional levels through plasmid overexpression is a pervasive strategy (Hernandez-Montalvo et al., 2003; Wang et al., 2006), it has several disadvantages, including metabolic burden and unexpected lateral effects. Modulation of galP and glk expression levels through plasmid overexpression or high strength promoter substitution cannot provide multiple combination of expression intensity for screening. Discovering a way to effectively modulate the transcription of the two genes to an optimal strength in combination is a pressing problem. We adopted MAGE to simultaneously regulate galP and glk expression levels (Wang H.H. et al., 2009). Using this approach, colonies with high PHB yields can be identified using Nile red dye staining.

After 16 rounds of MAGE modulation (Figure 3), recombinant strains were screened by Nile red staining. Recombinant strains with higher PHB production showed redder color. Screening and sequencing results are shown in Table 3. Using single colony color screening, we found that the RBS of both glk and galP genes were changed, and the amount of ssDNA (single string DNA) recombination of glk exceeded that of galP. This may be because the location of the glk gene is more susceptible to ssDNA recombination during genome replication. However, no recombinant was screened out in which the two genes were simultaneously mutated.

FIGURE 3

Figure 3. MAGE procedure. The red squares represent the cells, the black circles represent the ptkRED plasmid, and Exo, Bet and gam are the gene sequences of the enzymes on the plasmid. The yellow and blue circles represent the bacterial genome, with the red portion representing the target engineered gene sequence. Exo, exonuclease; Bet, phage recombination protein Bet; gam, host-nuclease inhibitor protein Gam.

TABLE 3

Table 3. Screening result of MAGE recombination strains.

Nineteen mutant strains were selected and transformed with pFF and pCAB, subsequently. Three batches fermentation of these 19 strains lead to the selection of strains in consideration of glucose consumption and PHB content, named EPPG-6, EPPG-16, EPPG-51, and EPPG-62 (Figure 4D). Then, we repeated fermentation using the four selected strains (Figure 4E). Fermentation results showed that after glucose transport system modulation, the DH-EPPG-6 strain had a recovered growth rate. The PHB yield reached 71.2% (mol/mol), which was 63.7% higher than that of the strain DH-EP. Then DH-EPPG-6 strain was renamed L-6, in which the wild type RBS sequence of galP was mutated to TGAAAGGGAAA.

FIGURE 4

Figure 4. Fermentation result of the engineered EP-bifido strains. (A) Growth curve of first batch selection. (B) Growth curve of second batch selection. (C) Growth curve of third batch selection. (D) PHB content and glucose consumption of these three batches selection. The blue columns represent PHB content and orange red broken line represents glucose consumption. (E) PHB content and yield of selected recombinants. The experiments were performed in triplicate and error bars indicate s.d. For mutant fermentation selection, strains were cultivated with M9 at 37°C, 150 rpm. (F) Growth curve of selected recombinants.

Expressing Heterogeneous Sugar Transporter to Reinforce Glucose Uptake

To further enhance the consumption of glucose, we compared the kinetic parameters of several transporters with their glucose transport capacity and energy consumption during glucose internalization and phosphorylation (Gosset, 2005). Because the transmembrane proton potential is a form of energy, the energy consumption of the glf sugar transporter from Zymomonas mobilis is comparable to that of the E. coli glucose-specific PTS (PTS^Glc). Compared with galP, the glf_zm transporter used less energy to produce a higher maximum velocity. Therefore, the high-rate, low-energy sugar transporter glf_zm was chosen to improve the glucose absorption capacity of engineered bacteria. Then glf_zm was inserted at the attP genomic site of strain L-6 using the CRIM plasmid system (Haldimann and Wanner, 2001), resulting the strain M-6. We deduced that glf integration was conducive to growth recovery in later growth stages. In Figure 5B, M-6 (pFFpCAB) showed a better growth curve than the control DH5α (pCDFpCAB). Simultaneously, as we expected, gross glucose consumption improved compared with L-6, increased from 16.2 to 20.4 g/L (Figure 5A). The glucose consumption of all engineered strains changed obviously after every modification step. PHB titer of M-6 improved significantly, from 4.82 to 5.81 g/L in comparison with that of L-6 (Figure 5D), and PHB content in M-6 strain reached 85.1 wt% (Figure 5E). The only drawback was that PHB yield of M-6 reached 68.1% (mol/mol) slightly decreased compared with L-6 (Figure 5E). In general, compared with parental strain DH-EP (pFFpCAB), the PHB titer and content improved 41.71 and 24.41% in M-6, respectively. And compared with the control DH5α (pCDFpCAB), the PHB content and yield of M-6 improved 61.9 and 141.7% in M-6, respectively (Figure 5). All the engineered strains produced some amount of acetate, M-6 and L-6 produced less acetate than DH-EP strain. We also calculated the acetate formation and glucose consumption normalized by residual cell mass (RCM).

FIGURE 5

Figure 5. The fermentation profile and PHB yield of all the engineered EP-bifido strains. (A) Glucose consumption. (B) Cell dry weight. (C) Acetate production. (D) PHB production. (E) PHB content and PHB yield. (F) Glucose consumption and acetate normalized by residual cell mass. The experiments were performed in triplicate and error bars indicate s.d. Strains were cultivated in M9 with glucose at 37°C, 150 rpm.

In order to confirm that the glucose consumption rates in our engineered strains are indeed improved, we calculated the specific growth rate and glucose utilization rates of DH-EP (pFFpCAB), DH5α-EPP (pFFpCAB), L-6 (pFFpCAB), and M-6 (pFFpCAB). After ptsG gene was deleted, the specific growth rate of DH-EPP decreased from 0.20 to 0.09 h^–1, and the glucose utilization rate decreased from 0.78 to 0.41 g L^–1 h^–1 (Table 4). After glf_zm integration based on L-6, the specific growth rate of M-6 (pFFpCAB) increased obviously from 0.28 to 0.50 h^–1, improved 42.8% compared to that of DH5α (pFFpCAB). The growth consumption rate recovered to 0.71 g L^–1 h^–1, 73% higher than DH-EP (pFFpCAB). M-6 and L-6 showed lower normalized glucose consumption. Thus M-6 and L-6 had improved PHB biosynthesis and PHB productivity since they produced less by-product acetate and consumed less glucose per residual cell mass (Figure 5F and Table 5).

TABLE 4

Table 4. Specific growth rates and glucose utilization rates of DH5α, DH-EP (pFFpCAB), DH-EPP (pFFpCAB), L-6 (pFFpCAB), and M-6 (pFFpCAB).

TABLE 5

Table 5. PHB productivity of the engineered PHB-producing strains.

We further examined the CO₂ release from the constructed EP-bifido strains. The total CO₂ release of DH5α-EPP (pFFpCAB) decreased to 32.5% compared to DH-EP (pFFpCAB) (Figure 6A). And the CO₂ emission of L-6 (pFFpCAB), M-6 (pFFpCAB) improved 177 and 332% compared to that of DH5α-EPP (pFFpCAB). We believe that the restoring growth contributed to the increased CO₂ release. The CO₂ yield of DH5α-EPP (pFFpCAB), L-6 (pFFpCAB), and M-6 (pFFpCAB) decreased to 16.9% (mol/mol), 74.4% (mol/mol) and 92.4% (mol/mol) compared to their controls, respectively (Figure 6B). The above data confirmed the recovery of growth after PTS system deficiency and the decreased CO₂ emission from the L-6 (pFFpCAB) and M-6 (pFFpCAB) strains.

FIGURE 6

Figure 6. Determination of CO₂ release. (A) Relative CO₂ emission and (B) CO₂ yield. Strains were cultivated in modified M9 medium containing 20 g/L glucose at 37°C and 150 rpm. CO₂ yield were calculated as mol/mol glucose × 100%. The experiments were performed in triplicate and error bars indicate s.d.

Discussion

As environmental problems intensify, carbon saving or carbon sequestration pathways have become a new focus for bio-manufacturing. Previously, we successfully constructed an efficient carbon-saving pathway in E. coli called the EP-bifido pathway. This pathway has been applied to the production of several compounds that use acetyl-CoA as a precursor. As a degradable material, PHB has great application prospects. While we believe that there is potential for further optimization of PHB production by the EP-bifido pathway. In this study, we knocked out the ptsG gene, a key glucose transporter of the PTS system that employs PEP as phosphate donor. The glucose consumption rate and cell growth were significantly reduced in the ptsG mutant under aerobic fermentation conditions. The deficiency in the PTS system dramatically impairs glucose uptake and causes growth restriction. It is speculated that the reason for growth restriction is not insufficient glucose uptake, but the subsequent decrease in glucose phosphorylation efficiency due to limited glucokinase activity (Steinsiek and Bettenbrock, 2012).

To overcome this growth hindrance, we optimized the RBS sequences of galP and glk genes, encoding glucose permease and glucokinase, respectively. Subsequently, we introduced the Z. mobilis glucose transporter, glf_zm, into the L-6 high-yield strain, and observed cell growth recovery. After optimization, PHB yield reached 71.9% (mol/mol) in L-6 strain. In the resulting strain M-6, the intracellular PHB content reached 85.1 wt%, and the titer reached 5.81 g/L. Previously, most studies have compensated for PTS knockout-induced inhibition of glucose uptake by overexpression of glk, and galP or by heterologous expression of glf (Snoep et al., 1994; Gosset, 2005; Lin et al., 2018). Instead, we applied MAGE technology to directly alter genomic glk and galP to optimize their expression (Gallagher et al., 2014). Meanwhile, the RBS library constructed using MAGE provided rich genotypes for subsequent screening of high-yield PHB strains. After glf_zm integration, recovered growth rate and glucose consumption was evident in strain M-6. Compared with parent strain DH-EP (pFFpCAB), the glucose consumption of M-6 increased 4.6 g/L, 29.1% higher than that of parent strain in Figure 5A. The PHB content and yield of strain M-6 improved compared with that of DH-EP(pFFpCAB). M-6 and L-6 showed lower normalized glucose consumption. Thus M-6 and L-6 had improved PHB production since they produced less by-product acetate and consumed less glucose per residual cell mass. We inferred that increased glucose uptake enhanced flux through EMP, which is supported by increased cell growth. The growth of DH-EP strain improved with decreased acetate formation in M-6 strain. The specific growth rate and CO₂ release data of constructed strains further confirmed our inference. Our study provided an efficient way for improving glucose absorption and total carbon conversion rate in artificial carbon-saving pathways by replacing PTS with other glucose transporters. It also describes an efficient screening strategy for MAGE ssDNA recombineering technology. The efficient utilization of carbon sources has been one of the determinant for high productivity in microbial fermentation. In the future, the effective allocation of carbon resources and the construction of effective strategies for balancing cell growth and product biosynthesis will still be the direction of metabolic engineering.

Data Availability Statement

All datasets generated for this study are included in the article/supplementary material.

Author Contributions

QW and QQ designed the work. YLi, YLu, and JX performed the experiments. ZS and YLi analyzed the ¹³C-MFA data. QQ and QL encouraged this project. YLi and QW wrote the manuscript. All authors read and approved the final manuscript. All authors contributed to the article and approved the submitted version.

Funding

This work was supported by grants from the National Key R&D Program of China (2019YFA0904900), the National Natural Science Foundation of China (31730003, 31670047, and 31770095), and Young Scholars Program of Shandong University and State Key Laboratory of Microbial Technology Open Projects Fund (M2019-11).

Conflict of Interest

The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.

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