Catabolic Division of Labor Enhances Production of D-Lactate and Succinate From Glucose-Xylose Mixtures in Engineered Escherichia coli Co-culture Systems

Introduction

Production of D-lactate (LA) and succinate (SA) from renewable carbohydrate feedstocks provides a sustainable and greener alternative to their petroleum-based production (Abdel-Rahman et al., 2013; Ahn et al., 2016; Es et al., 2018). LA and SA serve as two important monomers in the production of biodegradable plastics, including poly(butylene succinate) (PBS) and poly(lactic acid) (PLA), respectively. SA is largely produced via petroleum-derived maleic anhydride, and only a handful of plants producing bio-based SA currently exists (Jansen and van Gulik, 2014). Meanwhile, ∼95% of global LA production occurs via fermentation, being derived almost entirely from costly raw materials such as grain starch or sucrose from sugar cane, feedstocks that compete with the food chain (Okano et al., 2010; Abdel-Rahman et al., 2011). Alternatively, lignocellulose-derived sugars from non-food carbohydrates such as agricultural residues, forest products, or energy crops represent an attractive feedstock for producing bio-based plastics due to their increased abundance and sustainability, as well as lower cost (Lynd, 2017). The two most abundant sugars in most lignocellulosic biomass is glucose (a hexose, accounting for ∼30–50% dry weight) from the cellulose fraction and xylose (a pentose, constituting ∼20–35% dry weight) from the hemicellulose fraction (Nieves et al., 2015). Minute quantities of other fermentable sugars (i.e., arabinose, galactose, mannose) are additionally found in lignocellulosic biomass (Nieves et al., 2015).

For many native and engineered bacteria, the inability to efficiently co-utilize sugar mixtures in mineral salts medium at high catabolic rates (e.g., > 2 g L^–1h^–1 for each sugar) is due to a complex, global regulatory phenomenon known as carbon catabolite repression (CCR), which often results in incomplete and/or sequential sugar utilization. For instance, in Escherichia coli, this sequential sugar preference is controlled via the coordinated action of the global transcriptional regulator cyclic AMP (cAMP) receptor protein (CRP) along with a second regulator specific to the secondary sugars of interest, such as xylose. Activation of the requisite xylose catabolism operons (i.e., xylFGH and xylAB) requires both activated CRP (active when bound by cAMP) and XylR (regulator specific for xylose catabolism, active when bound by xylose) (Song and Park, 1997; Figure 1). When wild-type E. coli ferments glucose–xylose mixtures, for example, cAMP levels are low because abundant extracellular glucose leads to the active mode of the phosphotransferase system (PTS), increasing the abundance of unphosphorylated PTS components (IIA protein) and inhibiting the activity of adenylyl cyclase (AC; catalyzing cAMP synthesis). Xylose catabolism thus does not occur due to the lack of activated CRP and, as a result, initiates only after glucose is mostly utilized and phosphorylated IIA protein activates AC, leading to high cAMP levels (Figure 1).

FIGURE 1

Figure 1. Regulatory and catabolic pathways for glucose and xylose metabolism in E. coli. The primary mechanism for glucose transport in E. coli is through the phosphoenolpyruvate: sugar phosphotransferase system (PTS), including components EIIBC^Glc, EIIA^Glc, Hpr, and EI (encoded by ptsG, crr, ptsH, and ptsI, respectively). Under high glucose concentrations, glucose is transported via EIICB^Glc, leading to more abundant unphosphorylated EIICA^Glc that inhibits adenylate cyclase (AC) and lowers cAMP levels. Glucose-induced catabolite repression is mainly caused by low levels of cAMP which leads to non-functional CRP. Without CRP activation, the transcriptional activation of xylose catabolism pathways cannot be achieved. Under low glucose concentrations, AC is active due to the decreased amount of unphosphorylated EIICA^Glc, thus leading to increased cAMP levels and activated CRP. Both activated CRP and XylR (activated when bound by xylose) are required to activate the xylose catabolic operons, xylAB and xylFGH. Phosphorylated sugar intermediates enter glycolysis or PPP pathways for full degradation. GalP functions as an alternative non-PTS glucose transporter and glk encodes cytoplasmic glucokinase to phosphorylate glucose for further glycolysis. Glucose uptake systems including both PTS components and GalP as well as Glk and XylR indicated in red ovals are genetic engineering targets to construct sugar specialists. Abbreviation: AC, adenylate cyclase; CRP, cAMP receptor protein; PPP, pentose phosphate pathway; Glc, glucose; Glc-6P, glucose 6-phosphate; Xyl; xylose.

To date, several engineered microorganisms producing LA [e.g., lactic-acid bacteria (LAB), Saccharomyces cerevisiae, E. coli] and SA (e.g., Mannheimia succiniciproducens, Corynebacterium glutamicum, Bacillus strains) have been reported using various substrates (Grabar et al., 2006; Ishida et al., 2006; Wang et al., 2011; Litsanov et al., 2012; Awasthi et al., 2018). While different strains have their own unique advantages/disadvantages (e.g., ease of genetic manipulation, product tolerance, and other physiological benefits), from a bioprocessing perspective, it is desirable that it should also be capable of rapidly and simultaneously utilizing the substrate at high initial loadings (e.g., ≥ 100 g L^–1 total sugar). Under such conditions, E. coli has proven to be a particularly promising biocatalyst for the production of both LA and SA. In particular, via a combination of engineering strategies, E. coli strains have been developed to produce both LA and SA at high yields (>90%) and titers (>90 g L^–1) and maximum productivities (>1.0 g L^–1 h^–1) (Sawisit et al., 2015; Utrilla et al., 2016; Sievert et al., 2017). Despite these achievements, however, challenges still remain with respect to the efficient conversion of glucose–xylose mixtures.

Owing to unique features such as strain-specific specialization and metabolic modularity, the engineering and use of synthetic microbial communities represent a promising bioprocessing strategy (Zhang et al., 2015; Zhou et al., 2015; Camacho-Zaragoza et al., 2016; Jones et al., 2017), with the potential to surmount many limitations faced by traditional monocultures (Lu et al., 2019; Roell et al., 2019). Through catabolic division of labor, for example, engineered co-cultures have specifically emerged as an effective strategy for achieving efficient co-utilization of different mixtures of lignocellulose-derived sugars (Eiteman et al., 2008; Zhang et al., 2015; Chappell and Nair, 2017; Wang et al., 2019). Eiteman et al. (2008) first demonstrated the utility of this approach, engineering a co-culture composed of E. coli sugar specialist strains to co-utilize glucose–xylose mixtures (∼14 g L^–1 total sugars). This general strategy was later expanded upon by others to develop a three-member community of E. coli specialists to co-utilize a mixture of glucose, galactose, and mannose (∼7.5 g L^–1 total sugars) (Chappell and Nair, 2017). Most recently, meanwhile, our group engineered two different catabolically orthogonal co-culture systems (derived from wild-type E. coli W or ethanologenic E. coli LY180), each capable of co-utilizing 100 g L^–1 of a glucose–xylose mixture (2:1 by weight) in mineral salt media by simple batch fermentation (Flores et al., 2019). In this work, we further explore the utility of this strategy by applying analogous principles to engineer two unique co-culture systems composed of catabolically orthogonal E. coli strains for the production of LA and SA from glucose–xylose mixtures. In both cases, optimization of initial population ratios between each strain pair proved a key design variable toward achieving efficient conversion of the feedstock mixture along with high production metrics. This strategy of “population-level” tuning helps to alleviate biosynthetic burden while circumventing technical difficulties that would otherwise accompany the more traditional optimization of multiple catabolic pathways in a single strain.

Results and Disccusion

Construction of Catabolically Orthogonal Sugar Specialists for D-Lactate Production

TG114 (a derivative of E. coli KO11 and based on E. coli W) has previously been shown to produce LA at maximum volumetric productivity (2.88 g L^–1 h^–1), titer (118 g L^–1), yield (98%), and chiral purity (>99.9%) in mineral salts medium containing 120 g L^–1 glucose (Grabar et al., 2006). In spite of this, however, poor performance is apparent in sugar mixtures as a result of CCR (Supplementary Figures S1A–D). Specifically, when cultured using a 100 g L^–1 glucose–xylose mixture (2:1 by mass), TG114 utilized 88% of the provided glucose within the first 24 h and 100% by 48 h, but only 38% of the supplied xylose by 96 h, corresponding to only ∼80% total sugar utilization. LA was produced, meanwhile, at overall and maximum volumetric productivities (Q_LA) of 0.80 ± 0.01 and 2.6 ± 0.4 g L^–1 h^–1, a final titer of 77 ± 1 g L^–1, and yield (Y_p/s) of 0.96 ± 0.02 g g-total sugars^–1 (note: all reported yields based on total sugars consumed). To overcome the sugar co-utilization bottleneck experienced by TG114, a division of labor approach was used to construct a pair of complementary, catabolically orthogonal specialist strains, each capable of catabolizing either glucose or xylose but not both sugars (Supplementary Figure S2A). Specifically, a glucose specialist strain, TGglc, was constructed by deleting the xylose-specific transcriptional activator XylR (encoded by xylR) to inactivate xylose catabolism. A xylose specialist strain, TGxyl, was constructed by deleting the major components of glucose transport and its initial catabolism (i.e., ptsI, ptsG, galP, glk) (Figure 1 and Table 1). To further enhance xylose utilization of this specialist strain, wild-type XylR was also replaced with a mutant copy [P363S and R121C; denoted as XylR^∗ and reported to enable a stronger activation of the D-xylose catabolic genes (Sievert et al., 2017)].

TABLE 1

Table 1. List of strains and plasmids used in this study.

Consistent with their respective genotypes, TGglc and TGxyl each preferentially utilized only one sugar when fermented in mineral salt media supplemented with 66 g L^–1 glucose and 33 g L^–1 xylose (Figures 2A,B and Table 2). TGglc utilized 100% of the supplied glucose within 48 h (77% within the first 24 h, similar to TG114) and virtually no xylose. This resulted in a maximum Q_LA of 2.0 ± 0.1 g L^–1 h^–1 (overall, Q_LA was 0.68 ± 0.01 g L^–1 h^–1), final LA titer of 66 ± 1 g L^–1, and Y_p/s of 0.96 g g-total sugars ^–1 (Figures 2C,D and Table 2). In contrast, under the same conditions, TGxyl consumed just ∼80% of supplied xylose by 96 h and no glucose (Figures 2A,B). Growth of TGxyl, meanwhile, was significantly less than that of TGglc and TG114 [1.1 ± 0.1 g-dry cell weight (DCW) L^–1 compared to 2.7 ± 0.1 and 2.9 ± 0.2 gDCW L^–1, respectively]. While this difference is at least in part due to the lower energy yield of xylose relative to glucose, it is also possible that, since TG114 was originally engineered for and adapted in mineral salt media containing only glucose as carbon source (Grabar et al., 2006), it may have only gained mutations specifically tailored for glucose catabolism. Despite its slower growth rate and reduced biomass accumulation, TGxyl still produced LA at a final titer of 25 ± 1 g L^–1, Y_p/s of ∼0.99 g g-total sugars ^–1, and maximum Q_LA of 0.50 ± 0.08 g L^–1 h^–1 (Figures 2C,D and Table 2).

FIGURE 2

Figure 2. Fermentation of glucose–xylose mixtures (2:1 by mass) by lactate-producing sugar specialist strains. Concentrations of (A) glucose, (B) xylose, (C) D-lactate, and (D) OD_550nm measured in the fermentation broth for TGglc (closed circles) and TGxyl (open squares). All fermentations were performed in batch mode and in mineral salts media. Data points represent the arithmetic mean of three replicates, and the error bars represent one standard deviation.

TABLE 2

Table 2. Comparing the performance of individual E. coli sugar specialists and co-cultures during D-lactate (LA) and succinate (SA) fermentation.

Engineering and Optimizing a Synthetic Co-culture for Efficient Conversion of Glucose–Xylose Mixtures to D-Lactate

Given their promising performance metrics with respect to LA production and minimal cross-catabolic activities, TGglc and TGxyl were next used as complementary specialist strains with which to engineer a synthetic co-culture. To balance catabolic rates, simple titration of the initial inoculum ratio between TGglc and TGxyl (e.g., 1:1, 1:50, 1:100) while maintaining a constant total initial OD_550nm of 0.05 (the same initial OD_550nm as in monoculture fermentations) was performed. As shown in Figure 3A and Table 2, glucose was completely utilized within 48 h for all ratios (similar to TG144 and TGglc monocultures). However, as a result of tuning the initial population, initial volumetric rates of glucose utilization (Q_Glc) were subsequently reduced over the first 24 h in a manner proportional to the relative abundance of TGglc (2.4 ± 0.1, 0.82 ± 0.40, and 0.13 ± 0.02 g L^–1 h^–1 for ratios 1:1, 1:50, and 1:100, respectively), along with initial rates of biomass accumulation (Figure 3D and Table 2). The corresponding profiles of xylose fermentation (Figure 3B), meanwhile, revealed the opposite and expected effect with respect to xylose catabolism; increasing abundance of TGxyl in the initial inoculum improves xylose utilization. More specifically, at equal abundance (i.e., 1:1), total xylose utilization reached merely 22% by 96 h. This corresponded to 5% less total sugar utilization than by TG114 monocultures (75 vs. 80% total sugar utilization, respectively; Table 2). However, by tuning the initial inoculum ratio to 1:50, 2.6-, and 1.5-fold increases in xylose utilization (58% total xylose used) were realized relative to co-cultures with a 1:1 initial inoculum ratio and TG114 monocultures, respectively (Table 2). Owing to this significant increase in xylose co-utilization, final LA titers achieved by 1:50 co-cultures reached 84 ± 2 g L^–1 (∼11% higher than the 1:1 co-culture; Figure 3C), while still maintaining high overall performance metrics (Y_p/s of 0.96 g g-total sugars^–1, maximum Q_LA of 3.7 ± 1.1 g L^–1 h^–1; Table 2). Further increasing the relative initial abundance of TGxyl, 1:100 co-cultures then enabled further increased utilization of supplied xylose, in this case reaching ∼71% (Figure 3B). Moreover, total sugar utilized reached 91% by the end of the 96 h fermentation, achieving a final LA titer of 88 ± 1 g L^–1, Y_p/s of ∼0.97 g g-total sugars^–1, and maximum Q_LA of 2.5 ± 0.2 g L^–1 h^–1 (Table 2). Based on the promising trends observed with 1:50 and 1:100 co-cultures, additional tuning of the inoculum ratio to further increase the initial abundance of TGxyl was subsequently performed, in this case at both 1:500 and 1:1,000 (data not shown). However, no further performance enhancements were realized in terms of either total sugar utilization or LA production in such co-cultures, suggesting that the optimal initial inoculum ratio for TGglc:TGxyl exists at least close to 1:100. Thus, further improvement of this co-culture should next focus on enhancing the inherent properties of each individual strain; for example, increasing rates of xylose catabolism in sugar mixtures by TGxyl through adaptation and/or genetic engineering.

FIGURE 3

Figure 3. Fermentation of glucose–xylose mixtures (2:1 by mass) co-cultures composed of catabolically orthogonal lactate-producing specialist strains. Concentrations of (A) glucose, (B) xylose, (C) D-lactate, and (D) OD_550nm measured in the fermentation broth for TGglc:TGxyl co-cultures using an initial inoculum ratio of 1:1 (closed circles), 1:50 (open squares) and 1:100 (open triangles). All fermentations were performed in batch mode and in mineral salts media. Data points represent the arithmetic mean of three replicates, and the error bars represent one standard deviation.

LA production performance demonstrated by the 1:100 co-culture compares well to that of other co-cultures previously engineered for the same purpose, as well as those developed to produce other related fermentation products (Table 3). In particular, Eiteman et al. (2009) developed an E. coli co-culture composed of glucose and xylose specialists capable of co-utilizing and converting a sugar mixture (∼47 g L^–1 total sugar, ratio of glucose to xylose is 1.5:1 by mass) to LA (final titer of 32 g L^–1, Y_p/s of 0.68 g g-total sugars^–1) in a two-stage, aerobic–anaerobic process (Table 3). In this case, rather than tuning the initial population ratio, a sequential inoculation strategy was instead employed to balance the contribution of each specialist to the net catabolic activity, allowing more time initially for the xylose specialist strain to accumulate under aerobic conditions. Upon reaching the anaerobic phase, the population ratio in their co-culture was estimated as 2:3 glucose:xylose specialists, which similarly illustrates a need for increased abundance of the xylose specialist in this fermentation. In comparison to LA-producing monocultures, Sievert et al. (2017) demonstrated that substituting wild-type xylR with xylR^∗ (R121C and P363S; the same mutations used to develop TGxyl in this study) in TG114 enabled co-utilization of 50 g L^–1 glucose and 43 g L^–1 xylose (from 100 g L^–1 glucose–xylose mixture, initially 1:1 by mass) to 86 g L^–1 LA in mineral salt medium. While minor improvement in terms of sugar utilization was achieved using the present co-culture system, a unique advantage of this approach is the facile tunability that it provides. In this case, catabolic rates can be titrated to achieve optimal fermentation performance by altering initial inoculum ratios between the two specialists. This ability will likely be beneficial when utilizing feedstocks of varying compositions and can be extended beyond simply binary sugar mixtures.

TABLE 3

Table 3. Comparing the performance of different E. coli co-cultures engineered to convert glucose and xylose to fermentative products.

Finally, one intriguing observation associated with the developed LA co-culture system was that the volumetric rate of xylose utilization (Q_Xyl) was found to consistently and abruptly decrease in all co-cultures upon exhaustion of available glucose. For instance, as seen in Figures 3A,B, prior to glucose exhaustion, maximum Q_Xyl values were ∼0.35 ± 0.04, 0.44 ± 0.04, and 0.52 ± 0.05 g L^–1 h^–1 for 1:1, 1:50, and 1:100 co-cultures, respectively. However, following glucose exhaustion, Q_Xyl in the same co-cultures then dropped to just 0.034 ± 0.009, 0.062 ± 0.004, and 0.12 ± 0.02 g L^–1 h^–1. It is unlikely that LA or by-product toxicity is responsible for this behavior since the parent strain (TG114) has been shown to achieve LA titers up to 120 g L^–1, and almost no other side products are detected during its fermentation (Grabar et al., 2006). This observation possibly suggests that, although the two strains were engineered to be catabolically orthogonal, interstrain interactions certainly do occur throughout these synthetic co-cultures. The exact nature and extent of this behavior remain unknown, however, and warrant further investigation.

Construction of Catabolically Orthogonal Sugar Specialists for Succinic Acid Production

To further investigate the generalizable nature of this co-culture strategy along with sets of specific genetic modifications used to create each sugar specialist, the same methodologies were next analogously applied to SA production from glucose–xylose mixtures. In this case, the succinogenic strain KJ122 (a derivative of E. coli ATCC 8739) was used as the common parent for constructing the two sugar specialist strains: KJglc and KJxyl (Table 1 and Supplementary Figure S2). KJ122 was previously engineered and shown to ferment 100 g L^–1 glucose to SA (final titer of 82 g L^–1, overall Q_SA of 0.88 g L^–1 h^–1, Y_p/s of 0.90 g g-total sugars^–1) in mineral salts media (Jantama et al., 2008). Similar to TGglc, batch fermentation of KJglc also revealed virtually no xylose utilization (Figure 4B). In this case, glucose was completely utilized within 42 h at a maximum Q_Glc of 2.1 ± 0.1 g L^–1 h^–1, while SA was produced at a maximum Q_SA of 1.9 ± 0.1 g L^–1 h^–1. At this output, the performance of KJglc was similar to that of its parent strain, KJ122 (Figure 4A, Table 2, and Supplementary Figures S1A–D). Likewise, and as expected, KJxyl was unable to utilize glucose throughout the 120 h fermentation (Figure 4A), but utilized 87% of supplied xylose, leaving just 5 g L^–1 unused (Figure 4B and Table 2). With maximum Q_Xyl and Q_SA of 0.60 ± 0.06 and 0.69 ± 0.20 g L^–1 h^–1, respectively, overall performance of KJxyl was also similar to that of KJ122 (Supplementary Figure S1A).

FIGURE 4

Figure 4. Fermentation of glucose–xylose mixtures (2:1 by mass) by succinogenic sugar specialist strains. Concentrations of (A) glucose, (B) xylose, (C) succinate, and (D) OD_550nm measured in the fermentation broth for KJglc (closed circles) and KJxyl (open squares). All fermentations were performed in batch mode and in mineral salts media. Data points represent the arithmetic mean of three replicates, and the error bars represent one standard deviation.

Engineering and Optimizing a Synthetic Co-culture for Efficient Conversion of Glucose– Xylose Mixtures to Succinic Acid

KJglc and KJxyl were next combined to develop a synthetic co-culture for producing SA from glucose–xylose mixtures, again employing the same population-level tuning strategy in order to optimize sugar co-utilization. Based on the outcomes revealed for LA production, initial inoculation ratios of 1:1, 1:50, and 1:100 KJglc:KJxyl were first explored. As shown in Figure 5B and Table 2, total xylose utilization and Q_Xyl were similar for each of the 1:1, 1:50, and 1:100 co-cultures (each ∼87% and ∼0.67 g L^–1 h^–1, respectively) and close to that of the KJxyl monoculture. Meanwhile, however, total glucose utilization unexpectedly declined across this initial series of co-cultures (Figure 5A). For instance, compared to 1:1 co-cultures, total glucose utilization dropped by 80 and 94% in the 1:50 and 1:100, respectively; while all three co-cultures displayed reduced maximum Q_Glc relative to KJglc monoculture (Figure 5B and Table 2). Overall, total sugar utilization was 91, 39, and 31% for the 1:1, 1:50, and 1:100 co-cultures, respectively (compared to 71% for KJglc monocultures; Table 2), with the highest final SA titers reaching 84 g L^–1 ± 1 at the 1:1 ratio (at least two-fold greater than by 1:50 or 1:100) along with a maximum Q_SA of 1.3 ± 0.1 g L^–1 h^–1 (Figure 5C and Table 2). Interestingly, in contrast to the above LA co-cultures as well as our previous work (Flores et al., 2019), increased initial relative abundance of the xylose specialist did not result in enhanced xylose utilization or, in this case, improved production of SA (Figures 5B,C). This is likely because, in contrast to TGxyl, KJxyl displays much greater fitness, as demonstrated, for example, by its ability to accumulate twice as much biomass during monoculture fermentations [2.7 ± 0.2 gDCW L^–1 vs. 1.1 ± 0.1 gDCW L^–1 for TGxyl and 1.7 ± 0.1 gDCW L^–1 for LYglc1, a previously engineered ethanologenic xylose specialist (Flores et al., 2019)]. To test if it was in fact the relative activity of the glucose specialist that instead limited the overall performance of this SA-producing co-culture, an initial inoculum ratio of 2:1 KJglc:KJxyl was at last explored. While the 2:1 co-culture utilized glucose at a faster rate and consumed 100% of provided glucose by 96 h (compared to 44 h for KJglc monoculture and KJ122), total xylose utilization, on the other hand, dropped to just 46% overall (about half of that consumed by the 1:1 co-culture; Figure 5B and Table 2). Based on this outcome, it was determined that the optimal initial inoculum ratio for this specific co-culture was close to 1:1. Meanwhile, the finding that a unique optimum initial population ratio was required for the developed LA- and SA-producing co-cultures is not altogether surprising and likely reflects the fact that the relative fitness levels differ between the two strains that make up each pair.

FIGURE 5

Figure 5. Fermentation of glucose–xylose mixtures (2:1 by mass) co-cultures composed of catabolically orthogonal succinogenic specialist strains. Concentrations of (A) glucose, (B) xylose, (C) succinate, and (D) OD_550nm measured in the fermentation broth for KJglc:KJxyl co-cultures using an initial inoculum ratio of 1:1 (closed circles), 1:50 (closed dashed triangle), 1:100 (asterisk), and 2:1 (open squares). All fermentations were performed in batch mode and in mineral salts media. Data points represent the arithmetic mean of three replicates, and the error bars represent one standard deviation.

For comparison, Xia et al. (2015) previously developed an E. coli co-culture to convert glucose and xylose to SA via a two-stage, aerobic–anaerobic fed-batch process. Specifically, a mixture composed of ∼30 g L^–1 glucose and ∼10 g L^–1 xylose were first utilized aerobically for growth (producing no succinate), before then switching to anaerobic conditions to produce SA (∼15 g L^–1 glucose and ∼5 g L^–1 xylose were provided initially and then periodically added over 80 h; Table 3). Total sugar addition to this process over its 115 h duration was ∼100 g L^–1 (3:1 glucose:xylose by mass), and final SA titers reached ∼45 g L^–1. From a bioprocessing perspective, while this two-stage approach has proven to be effective, use of a process that can operate simple batch mode, such as the co-culture systems presented here, simplifies operation and control of the process. Similar to LA production, researchers have also engineered generalist strains to produce SA efficiently from sugar mixtures. For example, KJ122 further engineered to enhance conversion of a series of glucose–xylose mixtures (each 100 g L^–1 total with 1:1, 2:1, or 3:1 glucose:xylose by mass) to up to ∼84 g L^–1 SA using a combination of genetic engineering and adaptive laboratory evolution (Khunnonkwao et al., 2018). As discussed above, however, the current co-culture strategy is appealing due to its ability to facilitate effective catabolism of sugar mixtures through population tuning.

Overall, we have demonstrated the broad utility of engineering co-cultures composed of catabolically orthogonal E. coli strains for efficiently converting sugar mixtures into LA and SA, two important bioplastic monomers. Initial inoculum ratio was revealed to be an important design parameter for maximizing co-culture performance, the optimum value of which is unique to each specialist pair and can vary by even several orders of magnitude depending on relative phenotypic differences between member strains (Figure 6). Ultimately, by applying a population-level tuning strategy to balance rates of glucose and xylose co-utilization, both co-culture systems developed here were capable of fermenting a 100 g L^–1 glucose–xylose mixture at ∼91% conversion to either LA or SA at high rates and yields. This population-level tuning strategy was simple to implement experimentally and should similarly prove useful in other co-culture applications. Holistically, this work contributes to an improved understanding of the behaviors of synthetic microbial consortia as enhanced bioproduction platforms for renewable fuels and chemicals from non-food carbohydrates. Ultimately, however, the ability to elucidate and understand the nature and potential importance of interstrain interactions and/or metabolite exchanges (Herre et al., 1999; Ponomarova and Patil, 2015; Scott and Hasty, 2016) will likely be important to further optimize these and other co-culture systems.

FIGURE 6

Figure 6. Tuning the initial inoculum ratio enables enhanced bioplastic monomer production from glucose-xylose mixtures by co-cultures of catabolically-orthogonal specialist strains.

Materials and Methods

Strain Construction

All E. coli strains and plasmids used in this study are presented in Table 1. A list of primers used is presented in Supplementary Table S1. The xylose specialist strain (ΔgalP ΔptsI glk:kan^R xylR:xylR^∗) derived from KJ122 was initially found to grow poorly in media containing glucose–xylose and was accordingly adapted for improved growth under the conditions of interest. Growth was found to be significantly improved after performing just a single transfer, after which one clone, designated as KJxyl, was isolated. All chromosomal modifications were conducted using one- or two-step integration processes (Datsenko and Wanner, 2000; Sievert et al., 2017). Plasmid pXW001, containing a cat-sacB cassette, or strain T-SACK, containing a tetA-sacB cassette, were used as the PCR template to generate DNA fragments for primary integration into chromosomal sites of interest (Li et al., 2013; Sievert et al., 2017). Primary integration fragments contained the cat-sacB or tetA-sacB cassette flanked by 50-bp homology sequences from both upstream and downstream regions of the gene of interest. To eliminate the integrated cat-sacB or tetA-sacB cassette, providing markerless gene deletions, secondary integration fragments were generated containing 500-bp homology sequences from both upstream and downstream regions of the gene of interest, as generated via fusion PCR. Plasmid pKD46, expressing λ-red recombinase, was used to facilitate all chromosomal integrations via double-crossover recombination, as previously described (Datsenko and Wanner, 2000). During both primary and secondary chromosomal integrations, cultures were inoculated in a 250 ml flask containing 25 ml Luria Broth (LB), 50 g L^–1 arabinose, and 50 mg L^–1 ampicillin and incubated at 30°C with shaking at 150 rpm until the optical density at 550 nm (OD₅₅₀) of the cultures reached ~0.5. To prepare competent cells, cultures were subsequently centrifuged (5 min, 6,750 × g, 4°C), the supernatant was discarded, and the remaining cell pellet was resuspended in 20 ml of 4°C water. The described spin-wash cycle was repeated three times. On the last wash, all the supernatant was discarded except ~150–200 μl of the remaining supernatant which was used to resuspend pelleted cells. For electroporation, 40 μl of competent cells were combined with 100–200 ng of DNA. Following electroporation, cells were transferred to a sterile test tube containing 1 ml LB and incubated at 30°C for 4 h. Cells were then plated on LB plates containing the appropriate antibiotic. Colony PCR and Sanger sequencing were used to verify positive clones after selecting for appropriate antibiotic resistance during primary integration and sucrose insensitivity (10% w/v) and loss of antibiotic resistance during secondary integration.

Cultivation Conditions

Monoculture and co-culture batch fermentations were conducted in a pH (7.0)- and temperature (37°C)-controlled vessel containing 300 ml of modified AM1 mineral salt medium (Martinez et al., 2007; Yomano et al., 2009) containing twice the ammonium phosphate [38.8 mM (NH₄)₂H₂PO₄ and 15.1 mM (NH₄)H₂PO₄] and 67 g L^–1 glucose and 33 g L^–1 xylose (Flores et al., 2019; Martinez et al., 2019). pH was maintained by automatic addition of 6 M KOH for LA-producing cultures and a mixture of 6 M KOH and 3 M K₂CO₃ (1:4 ratio by volume) for SA-producing cultures, as previously described (Grabar et al., 2006; Jantama et al., 2008). From –80°C frozen stocks, strains were streaked onto AM1 agar plates supplemented with 100 mM MOPS and 20 g L^–1 glucose or 20 g L^–1 xylose. Agar plates were placed inside a sealed canister filled with argon gas and incubated at 37°C for 16–24 h. Seed cultures were grown in AM1 medium containing 100 mM MOPS, 10 g L^–1 glucose, and 10 g L^–1 xylose and incubated at 37°C with shaking at 120 rpm for ∼12–16 h. Cells were harvested by centrifugation (5 min, 6,750 × g, 4°C) and resuspended in 300 ml fresh media. All monoculture and co-culture fermentations were seeded using a total initial OD_550mn of 0.05 (∼0.022 gDCW L^–1).

Analytical Methods

Cell growth was quantified using a UV/Vis spectrophotometer (Beckman Coulter DU-730, Indianapolis, IN, United States). Sugar and product concentrations were determined by high-performance liquid chromatography (HPLC; Thermo Fisher Scientific and UltiMate 3000, Waltham, MA, United States) equipped with a refractive index detector. Analyte separation was performed using an Aminex HPX-87H column (Bio-Rad Laboratories, Hercules, CA, United States) maintained at 45°C and a mobile phase consisting of 5 mM H₂SO₄ flowing at a constant rate of 0.4 ml min^–1. External standards prepared in house were used to quantify substrate and product concentrations. All experiments were performed in at least triplicates, and the average and standard deviation are shown in figures and tables.

Data Availability Statement

The datasets generated for this study are available on request to the corresponding author.

Author Contributions

AF, DN, and XW designed the experiments, analyzed the data, and wrote the manuscript. AF constructed all strains and performed all experiments with the assistance of HC, RM, MO, EA, AG, and MM.

Funding

This work was supported by the start-up fund from Arizona State University (ASU) and ASU LightWorks. AF was supported by an IGERT-SUN fellowship funded by the National Science Foundation (Award 1144616). HC was supported by a Research Experience for Undergraduate (REU) grant (Award 1511637). RM was supported by WAESO LSAMP Bridge to Doctorate Fellowship.

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.

Acknowledgments

We thank Prof. Lonnie Ingram, formerly of the University of Florida, for providing strains TG114 and KJ122. We also thank Dr. Donald Court (National Cancer Institute, Center for Cancer Research) for the generous gift of E. coli W3110 variant T-SACK.

Supplementary Material

The Supplementary Material for this article can be found online at: https://www.frontiersin.org/articles/10.3389/fbioe.2020.00329/full#supplementary-material

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