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Efficient biosynthesis of (R)-mandelic acid from styrene oxide by an adaptive evolutionary Gluconobacter oxydans STA

Abstract

Background

(R)-mandelic acid (R-MA) is a highly valuable hydroxyl acid in the pharmaceutical industry. However, biosynthesis of optically pure R-MA remains significant challenges, including the lack of suitable catalysts and high toxicity to host strains. Adaptive laboratory evolution (ALE) was a promising and powerful strategy to obtain specially evolved strains.

Results

Herein, we report a new cell factory of the Gluconobacter oxydans to biocatalytic styrene oxide into R-MA by utilizing the G. oxydans endogenous efficiently incomplete oxidization and the epoxide hydrolase (SpEH) heterologous expressed in G. oxydans. With a new screened strong endogenous promoter P12780, the production of R-MA was improved to 10.26 g/L compared to 7.36 g/L of using Plac. As R-MA showed great inhibition for the reaction and toxicity to cell growth, adaptive laboratory evolution (ALE) strategy was introduced to improve the cellular R-MA tolerance. The adapted strain that can tolerate 6 g/L R-MA was isolated (named G. oxydans STA), while the wild-type strain cannot grow under this stress. The conversion rate was increased from 0.366 g/L/h of wild type to 0.703 g/L/h by the recombinant STA, and the final R-MA titer reached 14.06 g/L. Whole-genome sequencing revealed multiple gene-mutations in STA, in combination with transcriptome analysis under R-MA stress condition, we identified five critical genes that were associated with R-MA tolerance, among which AcrA overexpression could further improve R-MA titer to 15.70 g/L, the highest titer reported from bulk styrene oxide substrate.

Conclusions

The microbial engineering with systematic combination of static regulation, ALE, and transcriptome analysis strategy provides valuable solutions for high-efficient chemical biosynthesis, and our evolved G. oxydans would be better to serve as a chassis cell for hydroxyl acid production.

Background

An important challenge in the bio-manufacturing of high-value natural and unnatural chemicals is to develop green, efficient, and promising synthetic routes from cheap and readily available substrates. Epoxides are primarily from easily obtainable petroleum-based by-products and have broad applications in preparing pharmaceutical and fine chemicals [1,2,3]. Recently, epoxides have attracted much attention for hydrolyzing chiral vicinal diols to further synthesize unnatural compounds [4]. Our previous work had provided a self-sufficient cascade to biocatalytic epoxides to produce 1,2-amino alcohols [5].

The chiral (R)-mandelic acid (R-MA), as a useful chiral building block for the synthesis of aromatic drugs, is of crucial importance in the chemical and pharmaceutical industry [6,7,8]. Optically pure R-MA is an important intermediate for preparing many chiral drugs, including antitumors, antiobesity agents, antibiotics [9, 10]. In addition, MA also can be used to synthesize chiroptical materials [11,12,13]. Nowadays, R-MA is mainly produced by chemical synthesis with many by-products. Conversely, biosynthesis is an attractive alternative way to produce R-MA, which is non-toxic and has mild reaction conditions with high selectivity. It is an attractive and desirable way to produce R-MA using cheap styrene oxide as a substrate. However, the bioproduction of this valuable compound is still faced many challenges, including the lack of suitable catalysts and host strains for efficient synthesis reaction.

Recently, metabolic engineering in Saccharomyces cerevisiae and Escherichia coli and synthetic biology of multi-enzyme artificial cascades were used to synthesize R-MA [14, 15]. It is worth mentioning that they successfully produced R-MA from simple and readily available chemicals with high selectivity, whereas the yields are still not high. Among the cascade catalytic pathway described above, we noticed the accumulation of R-1-phenyl-1,2-ethanediol (R-PEG), which is probably because of the low expression and insufficient activity of alditol oxidase used to convert R-PEG to R-MA. In addition, an alcohol dehydrogenase and a phenylacetaldehyde dehydrogenase were assembled to biocatalyze S-PEG to S-MA [16], but there are few aldehyde dehydrogenases for the oxidation to R-MA.

The gram-negative obligate aerobic bacteria, acetic acid bacterium Gluconobacter oxydans, is famous for its stereo-selective incomplete oxidate sugars, alcohols, and polyols to the corresponding ketones and acids. As a wildly used industrial bacteria, G. oxydans has been successfully used to produce vitamin C, dihydroxyacetone, gluconic acid, and miglitol [17, 18]. Furthermore, it was reported that G. oxydans also was applied in oxidating R-PEG to R-MA by resting cells [19,20,21,22]. The conversion of the overwhelming majority of substrates and release of products do not need to transport the cell membranes, because the reactions typically occur in the periplasm using membrane-bound dehydrogenases, considerably improving the biosynthesis efficiency [23,24,25]. Hence, we selected G. oxydans as a host cell to construct a catalytic system for producing R-MA from styrene oxide.

However, studies have demonstrated that R-MA is toxic to G. oxydans and strongly inhibits to the oxidation reaction [19]. It may be a promising way to accelerate the catalytic efficiency and production by improving the R-MA tolerance of G. oxydans. Adaptive laboratory evolution (ALE) as an accessible and powerful approach in microbial engineering has become much more popular to obtain specially evolved strains with increased ability to survive under extreme conditions, inhibited metabolites, and toxic substrates or products [26,27,28,29,30,31]. Furthermore, ALE also successfully selected thermotolerant strains with improved growth and ethanol production in S. cerevisiae [32]. Recently, a 420-day adaptive laboratory evolution of G. oxydans was applied, resulting in a highly improved conversion efficiency of non-glucose sugars to sugar acids [33]. All the cases indicated that ALE is a powerful and efficient strategy to push microbe breakthrough the limit to synthesize toxic compounds.

In this study, we initially constructed an efficient catalytic system for producing R-MA from styrene oxide by heterologous expression of SpEH with a new screened endogenous strong promoter in G. oxydans (Fig. 1). Followed by the ALE strategy, an evolved G. oxydans named STA with enhanced R-MA tolerance ability was isolated and characterized. Then, we used transcriptome analysis of wild-type strain and STA to study their genetic mechanisms of the STA’s improved R-MA tolerance. Multiple vital genes involved in transcript levels changes were investigated, among which AcrA was confirmed to be essential for R-MA tolerance, STA-ΔacrA cannot even survive under a low concentration of R-MA. The evolved G. oxydans STA showed great potential for highly efficient R-MA production.

Fig. 1
figure 1

Scheme of bioproduction of R-MA from styrene oxide with recombinant G. oxydans 621H expressing epoxide hydrolase (SpEH) from Sphingomonas sp. HXN-200

Results and discussion

Developing a biocatalytic cascade and screening new strong promoters for R-MA production in G. oxydans

To construct a biosynthesis cascade to product R-MA from styrene oxide, epoxide hydrolase (SpEH, GenBank ID: ANJ44372.1) from Sphingomonas sp. HXN-200 [5, 34] was chosen as the first step for hydrolysis of styrene oxide into R-PEG. In addition, G. oxydans, a famous non-pathogenic and safe microorganism, has shown strong incompletely oxidize capacity to produce alcoholic acid including R-MA. Thus recombinant G. oxydans with heterologous expressing SpEH was constructed for highly efficient R-MA production from bulk chemical styrene oxide.

In synthetic biology, promoters and ribosome binding site are critical in controlling protein expression and gene regulation [35,36,37]. As strong promoters are essential for enhancing the expression of specific genes, employing a suitable and strong promoter is very important for spEH. However, the alternative constitutive strong promoters applied in G. oxydans 621H are still constrained. Thus, we aimed to screen out and identify strong endogenous promoters from G. oxydans to optimize the expression of SpEH.

Nowadays, numerous biological promoter engineers have been developed to model and design promoter libraries or screen strong endogenous promoters directly from the genome [38]. A range of studies have clarified that it is an accessible strategy to mine strong constitutive promoters based on RNA sequencing data. 25 genes with constitutive strong promoters in Methylotuvimicrobium buryatense 5GB1 were identified, relying on whole genome and RNA-sequencing experimental data [39]. It was also reported that in G. oxydans WSH-003, a few strong promoters were obtained through RNA-sequencing data, and with the strongest promoter P2703 expressing SDH, the titer of 2-keto-l-gulonic acid increased distinctly [40].

In RNA-sequencing data, the promoters of genes with high fragments per kilobase million (FPKM) values may be potentially strong. First, we performed RNAseq analysis on G. oxydans 621H, relying on transcriptome results of G. oxydans, the 10 top FPKM values of genes were chosen (Fig. 2a, Additional file 1: Table S3). To evaluate the strength, all the 10 putative promoters (500-bp upstream fragments), as well as the reported strong promoters Pdnak and PtufB from G. oxydans [41, 42] fused with egfp gene (GenBank ID: AAK08507.1) were ligated to pBBR1MCS-2 and transferred into G. oxydans. By assaying the fluorescence intensity, seven strong promoters were identified compared to the control, including P02805, P09400, P04650, P12780, P04000, P04750, and P10190. Furthermore, the green fluorescence also was observed (Fig. 2b). Then, we heterologous expressed SpEH in G. oxydans 621H with these new promoters. The expression results of SpEH were displayed by SDS–PAGE and their crude enzyme activities (obtained from the same growth and cell density) also were detected (Fig. 2c, d). It can be clearly seen that P12780 had the highest expression and the activity was higher than P02805 and P04650 for 5.5 and 1.8 times, respectively. The results indicated that the fluorescent protein's intensity can only illustrate the strength of promoters to a certain extent and cannot accurately represent the expression level of a specific protein [43, 44]. As P12780 was the most suitable promoter for the expression of SpEH in G. oxydans (WT-speh), it was used for the transformation of styrene oxide into R-MA and the original promoter of pBB vector was used as control (WT-control-speh). Compared to 7.36 g/L R-MA of the control, WT-speh got better production of 10.26 g/L (Fig. 2e).

Fig. 2
figure 2

a FPKM value of 10 top strongly transcribed genes of G. oxydans 621H. b Strength of screened promoters evaluated with eGFP as reporter and the microscope pictures of P02805, P09400, P04650 and P12780. c Relative activity of SpEH. SpEH were expressed with screened and reported promoters. The enzyme activity of SpEH controlled by Plac was set to 100% and its enzyme activity was 5.69 ± 0.26 U/mL. ****P < 0.0001. d SDS–PAGE of SpEH expression strains with the screened promoters. Lane M: protein marker; Lane 1: whole cell protein of G. oxydans 621H without overexpressing SpEH; Lanes 2–11: whole cell protein of recombinant G. oxydans strains with SpEH expressed by Plac, Pdnak, PtufB, P12780, P04000, P04750, P10190, P09400, P02805, P04650. e Biotransformation time course of styrene oxide to R-MA of WT-speh and WT-control-speh cells. f Growth curves for G. oxydans 621H under 0, 1, 2, 3 and 4 g/L R-MA

ALE of G. oxydans and phenotypic characterization of the evolved strain

As it was reported that R-MA was toxic to G. oxydans, we then verified its survivability to R-MA. By analyzing the growth curve, the tolerance of G. oxydans 621H to different concentrations of R-MA was determined. The growth rate delayed obviously with 3 g/L R-MA and the cells cannot grow when cultured with 4 g/L R-MA (Fig. 2f). Apparently, G. oxydans was very sensitive to R-MA. Typically, the capacity to tolerate high-concentration product is a prospective characteristic for high production of target compounds [45]. To further improve the production of R-MA, the ALE strategy, an efficient approach to generating strains with desired phenotypes under selection pressure, was performed to enhance R-MA tolerance in G. oxydans. As shown above, the cell growth of G. oxydans was affected even with very low R-MA concentration. Thus, we determined the starting point for ALE in a much lower concentration of 0.25 g/L R-MA. The wild-type G. oxydans were cultured for 24 h, then transferred into a fresh medium with 0.25 g/L R-MA and 5% inoculation volume. After incubation of 24–48 h, at log phase, these bacteria were transferred into a fresh medium containing 0.5 g/L R-MA. Repeat these transfers every time with 0.25 g/L R-MA increased (Fig. 3a). As the increase of the concentration, adapted G. oxydans strains need much more time to grow to log phase, at that time, we cultured the strains in the same R-MA concentration more times to improve the cell stability. The final concentration of R-MA was 6 g/L; after screening, the evolved strain named STA was isolated. To assess the genetic stability of STA, we transferred log-phase cells into a fresh medium without R-MA every 24 h for 30 days. At the last time of transfer, 6 g/L R-MA was contained in the culture medium and STA can grow as before which indicates that the R-MA tolerance of STA can be stably inherited (data not shown).

Fig. 3
figure 3

Adaptive laboratory evolution of G. oxydans to improve R-MA tolerance. a Schematic diagram of adaptive evolution. The original strain was G. oxydans 621H (WT). b Spot assays in G. oxydans WT and STA with 0 g/L, 3 g/L and 6 g/L R-MA. c Biotransformation time course of styrene oxide to R-MA of WT-speh and STA-speh cells. d Measurements of cell shape and length in wild-type G. oxydans and adapted strain STA

To probe the phenotypic characterization, the survival assay was used between G. oxydans WT and STA. STA can remain viable in the plate with 6 g/L R-MA but the wild-type strain had no capacity to survive (Fig. 3b). As P12780 was the most suitable promoter for expressing SpEH, we then transformed the recombinant plasmid pBB-P12780-speh into STA (STA-speh). Recombinant strains were subsequently used to transform styrene oxide into R-MA (Fig. 3c). It can be clearly seen that STA-speh showed better catalytic ability, which can produce14.06 g/L R-MA but WT-speh 10.26 g/L. Most importantly, conversion rate increased from 0.366 to 0.703 g/L/h. In addition, the expression levels of SpEH in these two strains were comparable and their enzymatic activities were almost the same (Additional file 1: Fig. S1).

Since SpEH was expressed intracellular, styrene oxide needs to be transferred to the intracellular to be hydrolyzed into R-PEG, while R-PEG also needs re-transmembrane to periplasmic space to be further oxidized by membrane-bound alcohol and aldehyde dehydrogenase to R-MA. Hydrophobic substrate styrene oxide conversion to R-MA requires two transmembrane operations in this biotransformation cascade. Thus, it would be very important to study cell characteristics for the STA strain to understand how the catalytic efficiency was improved after ALE strategy. Previous studies have certified that the membrane properties such as permeability, hydrophobicity, and integrity of evolved strains were found to be contributing to the increasing tolerance [46,47,48]. Compared to the wild-type strain, the evolved carboxylic acids tolerant E. coli strain with increased membrane rigidity and decreased fluidity was proved to have a fivefold increase in titer [49]. Initially, their morphologies were examined by scanning electron microscopy. In control, STA as well as the wild-type strain was both grown in fresh medium, their cells were of short rod shape, whereas STA cells were much less and shorter than the parent one (Fig. 3d). In all probability, the membrane properties of STA have changed compared to the wild-type strain.

We first investigated the inner and outer membrane permeability of the parent strain and STA assessed by hydrophilic probe propidium iodide (PI) and hydrophobic probe N-phenyl-1-naphthylamine (NPN) uptake analysis. As shown in Fig. 4a, b, STA exhibited a decrease in the fluorescence intensity of NPN with almost 50% and its PI absorption factor was only one-quarter of the wild-type strain, indicating that STA had a poor permeability membrane. PI emit a strong fluorescence signal when they transport into cells and bind to nucleic acids. As a result, PI also can serve as a probe to investigate membrane integrity by flow cytometer. The ratio of PI-stained cells of the wild-type strain was 84.2%, much higher than STA (Fig. 4c), which signified that STA had increased the membrane integrity. Interestingly, improved membrane integrity was shown to enhance the fatty acid tolerance and the final titer in E. coli [50].

Fig. 4
figure 4

Membrane integrity, permeability and hydrophobicity analysis of G. oxydans WT and the adapted strain STA. a NPN fluorescence intensity analyses of outer membrane permeability in WT and STA. b Inner membrane permeability change of propidium iodide (PI) uptake factor in WT and STA. c Flow cytometry analyses of membrane integrity in WT and STA. Cells were stained with PI. d Membrane hydrophobicity was changed in WT and STA. *P < 0.1. **P < 0.01. ***P < 0.001

Membrane hydrophobicity was another critical characteristic for cell viability and bioconversion activity. The STA strain had a percentage of adhesion of 21.0% relative to the control of 7.9%, which represented that the adaptive evolution of G. oxydans had significantly improved the membrane hydrophobicity (Fig. 4d). High cell surface hydrophobicity helped to against multi environmental stressors and reduce the distance of cell to hydrophobic substrate for the enhancement of transport rate [51, 52]. In summary, STA had worse membrane permeability and better membrane integrity, most importantly, the membrane hydrophobicity had increased. These membrane characteristics changes provide new insights into the understanding of R-MA tolerance and increasement of catalytic efficiency by STA.

Global transcriptome analysis and whole-genome sequencing of G. oxydans WT and STA

The differentially regulated genes in transcriptional levels were crucial factors for analyzing the cellular processes [53, 54]. To further explore the molecular mechanisms that accompanied R-MA tolerance of STA, transcriptome analysis was conducted to compare global gene expression in wild-type G. oxydans and STA under 0 g/L or 3 g/L R-MA condition. Comparative transcriptome data of wild-type G. oxydans with/without R-MA showed that the expression levels of 60 genes were significantly upregulated, while 192 genes were significantly downregulated at least twofold. By contrast, 58 genes upregulated and 209 genes downregulated at least twofold in STA (Fig. 5a, b). Only 143 commonly regulated genes are involved in wild-type G. oxydans and STA for the response to R-MA, which indicated that there must be some important genes regulated in STA relative to the tolerance of high R-MA concentration.

Fig. 5
figure 5

Transcriptome analysis of G. oxydans WT and STA. a Left side displays the gene expression differences of G. oxydans WT under normal and 3 g/L R-MA condition. The right side displays the gene expression differences of the adapted strain STA under normal and 3 g/L R-MA condition. X-axis represents the logarithmic conversion value of gene expression in wild type strain (left side) or adapted strain (right side). Y-axis represents the log2-transformed value of expression change folds. Classification of genes with different functions are represented by different color shapes as indicating. Others representative genes are not part of the indicated classification. b Venn diagrams showing the regulated gene numbers between G. oxydans WT and STA under 0 g/L R-MA and 3 g/L R-MA conditions (left side) and the regulated gene numbers between G. oxydans WT and STA in response to 3 g/L R-MA (right side). Six common regulated genes were depicted in the middle

The regulated genes in STA relative to those in WT were analyzed under normal and 3 g/L R-MA treatment conditions. As shown in Fig. 5b, common regulated genes were identified in G. oxydans WT and STA. Among these regulated genes, the multiple antibiotic resistance regulator family (MarR) gene and fusaric acid resistance protein family (FUSC) gene were upregulated by 7.57-fold and 6.30-fold in STA compared to the wild-type strain in normal condition. Similarly, these two genes also were upregulated when the wild-type strain was cultured with 3 g/L R-MA condition. Notably, MarR family transcriptional regulator is known for regulating diverse cellular responses and physiological processes [55]. Another two genes, encoding AcrA (efflux RND transporter periplasmic adaptor) and AraC family transcriptional regulator, were up-regulated in STA under 3 g/L R-MA condition. In wild-type strain, AraC regulator also was upregulated when facing 3 g/L R-MA, while AcrA was not regulated significantly. We also observed GltD (NAD(P)-dependent oxidoreductase) and GltB (glutamate synthase large subunit) genes were upregulated in STA compared to WT without R-MA, on the contrary, they all downregulated when STA was cultured with 3 g/L R-MA.

To identify genetic mutations contributing to the improved tolerance of R-MA, whole-genome sequencing was performed on the evolved strain STA, relative to the published sequence for wild-type G. oxydans 621H. STA carrying a large number of mutations and all the mutations including single nucleotide variations (SNVs) and nucleotides insertion-deletion (InDel) were listed in Additional file 2: Table S4-1. Among the mutation genes, there were two nonsynonymous mutations in the coding regions of GltB and MarR family transcriptional regulator (their mutations were further identified by gene sequencing and listed in Additional file 2: Table S4-2), which had also been reported to be related to cellular physiological processes, these processes showed response to the extreme environment or associating with the stress or antibiotics resistance. Most importantly, these two genes also were upregulated significantly in response to R-MA condition. MarR family transcriptional regulator has been shown to regulate diverse cellular processes, including conferring resistance to antibiotics, organic solvents, and virulence [56]. The glutamate synthase GltB was proved to be involved in the biofilm formation as well as the oxidative stress tolerance in Listeria monocytogenes [57].

Key genes that contribute to R-MA tolerance of G. oxydans STA

To study the contribution of the genes mentioned above, single-knockout strains of marR, fusc, gltD, gltB, acrA and araC were constructed in STA. The cell growth was determined in normal medium. There are no significant growth differences between STA and STAΔacrA, while deletion of other genes was slightly detrimental to cell growth (Fig. 6a). The growth curves under 4 g/L R-MA stress were investigated afterward. STAΔacrA have no capacity to survive just like wild-type G. oxydans. While all others had a delayed log phase and declined final cell density compared with the control (Fig. 6b). Knockout GltB increased the growth ability of STA under 4 g/L R-MA condition. To directly display the impact of these genes, the single-knockout strains were spotted and grown on culture plates with 0, 3 and 6 g/L R-MA. Delete marR, fusc, gltD, acrA and araC caused significant growth defects in the presence of 6 g/L R-MA compared to STA. Notably, different with other strains can grow normally at 3 g/L R-MA stress condition, the growing vitality of STAΔacrA had been greatly inhibited. We overexpressed the six genes in its corresponding knockout strains for further assessing their functions. As shown in Fig. 6c, five strains recovered the tole-rant phenotype, on the contrary, overexpress GltB caused a growth defect in 6 g/L R-MA stress. Clearly, the ability of STA to tolerant high-concentration R-MA required the interaction of multiple genes. Furthermore, as STA had changed the membrane properties compared to wild-type strain, we also explored the membrane properties of STA strains. As shown in Additional file 1: Fig. S2, compared to STA, STAΔgltB had better membrane permeability and STAΔgltD had worse membrane permeability. The membrane integrity and hydrophobicity of the strains was nearly the same.

Fig. 6
figure 6

Growth in G. oxydans STA of different gene deletions to test their contribution for R-MA tolerance. a Growth curves of G. oxydans STA and its gene-deletion strains under normal condition. b Growth curves of G. oxydans STA and its gene-deletion strains in the presence of 4 g/L R-MA. c G. oxydans STA and its gene-deletion strains were spotted on solid medium under 0 g/L, 3 g/L and 6 g/L R-MA condition

MarR and AraC as transcription regulators both were proved to regulate the expression of diverse genes related to stress and virulence response [58, 59]. AraC family regulator YdeO enhanced the acid and the multi-drug resistance in E. coli [60]. Another key gene was gltD, which altered the critical biofilm properties for environmental adaptation [61]. We also noticed that only deletion of AcrA led to significant growth defect with 3 g/L R-MA, which indicates that AcrA may play the most vital role in the tolerance of STA to R-MA. Consequently, we decided to focus on AcrA for further evaluation. AcrA belongs to RND efflux pumps, which have an important contribution to antibiotic resistance and microbial environmental adaptability in bacteria [62, 63]. Then, further analysis was performed to test whether AcrA had associated with other phenotypes. Surprisingly, the evolved strain STA showed higher growth rate than the wild-type G. oxydans under osmotic and low-pH stress (Fig. 7a). The AcrA knockout strain of STA completely lost the ability to survive under pH 3 condition and the osmotic tolerance also greatly reduced with 75 mM NaCl. To further verify the functions, it also was overexpressed in wild-type G. oxydans. Interestingly, G. oxydans/acrA exhibited improved tolerances in these stress conditions. In addition, all strains had the highest growth rate when none extreme factor was present, indicating that the normal growth of G. oxydans does not depend on AcrA.

Fig. 7
figure 7

Contribution of AcrA for G. oxydans WT and G. oxydans STA in cell growth under different environmental stress and final R-MA production. a Growth characterizations of WT, STA and AcrA associated strains are represented by the maximum specific growth rates (h−1). Right bar indicates the color-scale of the growth rate. b Transformation of styrene oxide into R-MA by WT, STA and AcrA associated strains with SpEH or SpEH co-expressing with AcrA

Validation the role of AcrA in R-MA production

AcrA, an RND efflux transporter, was reported to be a multidrug transporter for extrusion of a broad range of compounds in gram-negative bacteria. It also supports bacterial adaptation in the absence of different niches [64, 65]. Through inhibited RND pump, the drug susceptibility of E. coli was enhanced [66]. It also reported that an RND transporter upregulated in ALE-derived Pseudomonas putida for toluene tolerance [67]. In this study, when G. oxydans STA suffered with 3 g/L R-MA, the transcriptional levels of acrA were upregulated by 2.2-fold. In addition, compared to wild-type strain in 3 g/L R-MA condition, acrA was upregulated by 3.9-fold. Nevertheless, it was only 1.3-fold upregulation in the case of normal condition as STA compared to WT. Considering the critical function of AcrA in STA when facing environmental pressure, it could be practical to further improve the R-MA production by enhancing AcrA expression. Then, we coexpressed AcrA and SpEH in G. oxydans strains, and not only the final production of R-MA increased, the conversion rate also was improved. Most importantly, the R-MA production was further improved to 15.70 g/L by the evolved strain (Fig. 7b), which was the highest obtained from styrene oxide reported thus far.

Conclusions

In this study, G. oxydans was first used as a host cell for expressing SpEH to produce R-MA from bulk industrial chemical styrene oxide. After improving the R-MA tolerance of G. oxydans 621H by adaptive laboratory evolution together with the screened new strong promoter P12780 for enhancing SpEH expression, the production increased by 1.92-fold (from 7.36 to 14.06 g/L) and the conversion rate greatly improved from 0.366 to 0.703 g/L/h. We also described the membrane phenotype changes of the adapted G. oxydans STA, including better membrane integrity and increased membrane hydrophobicity, which may directly relate to the improved catalytic efficiency of organic substrate styrene oxide. Genomic sequencing and transcriptome analysis revealed that multiple key genes involved in enhancing R-MA tolerance. Finally, the R-MA production was further improved by an engineered G. oxydans STA. This study indicated that G. oxydans would be a promising host for the production of α-hydroxy acids from epoxides and its excellent ability to stereo-selective incomplete oxidation idols to the corresponding acids could be used to the maximum extent. In addition, ALE strategy combing with the comparative omics studies would be a valuable tool for enhancing chassis cell characteristics and guiding further metabolic engineering directions for high-value chemical production.

Materials and methods

Strains, media, and culture conditions

The G. oxydans strains used in this study are listed in Additional file 1: Table S1. G. oxydans cells were grown in the medium containing 8% sorbitol, 2% yeast extract, 0.1% KH2PO4, 0.05% MgSO4, 0.01% glutamine and incubated at 30 °C with shaking at 200 rpm. E. coli JM109 as host cell was used for plasmid construction and amplification and routinely grown at 37 °C in LB medium (0.5% yeast extract, 1% tryptone, 1% NaCl). 50 µg/mL kanamycin and 90 µg/mL gentamicin were used for selecting recombinant plasmids.

Construction of recombinant strains

The egfp and speh genes kept in our lab were amplified by PCR. All the screened potential promoters and the reported PtufB and Pdnak were amplified by PCR with G. oxydans 621H genome as the temple. The sequences of primers used for engineering recombinant plasmids are listed in Additional file 1: Table S2. The amplified promoter fragments were ligated with the corresponding egfp and speh genes, and inserted into the Hind III and Xho I site of pBBR1MCS-2. All the ligated productions were transformed into E. coli JM109 and followed by DNA sequencing to confirm the ligation results. Then, the engineered vectors were transformed into G. oxydans. The endogenous genes marR, fusc, gltD, gltB, acrA, and araC in G. oxydans STA were deleted by homologous recombination. We amplified their upstream and downstream homology arm fragments from genomic DNA of G. oxydans STA and ligated them with the marker gene of KAN amplified from pBBR1MCS-2. These fusion fragments were directedly introduced into G. oxydans STA, following which kan-resistant transformants were selected. Their genes were amplified and inserted into pBBR1MCS-5 using Gm antibiotics to select recombinant plasmids and then transformed into the corresponding single-knockout strains.

Adaptive laboratory evolution experiments

A G. oxydans 621H colony was inoculated into a 10 mL medium to culture about 24 h to the logarithmic phase. Then, transferred into 50 mL fresh medium containing 0, 1, 2, 3 and 4 g/L R-MA, respectively, monitored their growth by measuring the cell density at OD600. For the adaptive evolution experiments, the strategy of inoculating G. oxydans with gradually increasing the concentration of R-MA, and the initial concentration was 0.25 g/L. After cultivating to the log phase, the cultivation was transferred into the fresh medium with an increasing concentration of R-MA by 0.25 g/L each time at 5% inoculation volume. After a long term of adaption, the adaptive strains can survive in the medium containing 6 g/L R-MA, and we screened the single colony by plating on the plates with 6 g/L R-MA and named G. oxydans STA. To verify the genetic stability of G. oxydans STA, we cultured the single colonies of wild type G. oxydans and STA to log phase and then transferred them into fresh medium without R-MA every 24 h. After inoculating for 30 days, the cultivations were into fresh medium containing 6 g/L R-MA to observe their growth.

Spot assays and cell growth assays

G. oxydans was cultivated to logarithmic phase then diluted to an absorbance at 600 (OD600) of 2.0 in fresh medium, then aliquots of tenfold serial dilutions (4 µL) were spotted onto sorbitol plates containing no R-MA or indicated concentrations of R-MA. The cells were inculcated for 3 days in 30 °C.

G. oxydans strains were inoculated into 10 mL medium to culture about 24 h to the logarithmic phase and then transferred into 50 mL fresh medium containing 0, 1, 2, 3 and 4 g/L R-MA, respectively. We recorded the OD600 values at regular time intervals.

Transcriptome analysis and whole-genome sequencing

After the ALE assay, the endpoint colony of STA was selected for transcriptome analysis. G. oxydans WT and G. oxydans STA cells were cultured to a same OD600 of 2.3, then the cells were collected, rapidly frozen by liquid nitrogen. RNA extraction and transcriptome sequencing were performed by GENEWIZ Biotech Co., Ltd. (Suzhou, China). All differentially expressed genes were determined GENEWIZ (Suzhou, China). All differentially expressed genes were determined by q-value ≤ 0.05 and |log2ratio| of ≥ 1 (Additional file 2: Table S4). The genome of G. oxydans 621H (NC_006677.1) was used as the reference [68].

Then, a colony of STA was selected for whole-genome sequencing. 100 ng genomic DNA was randomly fragmented by sonication (Covaris S220) to a size of less than 500 bp. Then, end repairing, A-tailing and adding adaptors were treated to these fragments using End Prep Enzyme Mix. After amplification and purification, the products were validated using an Agilent 2100 Bioanalyzer. A PacBio sequencing library was constructed and then sequenced using the Sequel II sequencing platform. Based on de novo analysis, mutations of insertions, deletions, and single nucleotide mutations were identified with the wild-type G. oxydans 621H genome sequence as reference.

Fluorescence intensity assay and enzyme activity assays of SpEH

G. oxydans strains carrying the eGFP express plasmids of different promoters were cultivated in the logarithmic phase, collected and washed with 0.2 M PB buffer (pH 7.0) and resuspended in PB buffer at an appropriate concentration. The cell fluorescence was measured using Gen5 Data Analysis Software (BioTek, USA) at an excitation of 488 nm and an emission of 509 nm upon measuring 96-well plates. The normalized activity of eGFP was defined as the ratio of the fluorescence unit (RFUs) divided by the absorbance at 600 nm.

G. oxydans strains were cultivated to a same cell density in log phase, harvest, washed and resuspended with phosphate buffer (PB, 200 mM, pH 7.0) to be sonicated under the ice bath to obtain the crude enzyme solution and prepared a 0.2 M ethylene oxide substrate solution in methanol. 850 µL PB buffer mixed with 100 µL crude enzymes were placed at 35 °C for 5 min. The reaction started by adding 50 µL substrate solution and incubated for 10 min. The reaction was terminated by being treated in a boiling water bath for 10 min. The enzymic activity of SpEH was analyzed using high-performance liquid chromatography (HPLC). One unit of SpEH activity was defined as the amount of enzyme needed to hydrolyze ethylene oxide to produce 1 μmol 1-phenyl-1,2-ethanediol (PEG) per minute.

Biotransformation procedure to convert styrene oxide to R-MA with resting cells of G. oxydans strains

The SpEH expression strains of G. oxydans were cultured in 10 mL medium containing 50 µg/mL kanamycin and then transformed into 100 mL medium for 30 h to reach the logarithmic phase. The cells harvested by centrifuge (8000 rpm, 4 °C, 5 min) and washed twice, then resuspended in PB buffer. The fresh cell density of the biotransformation mixture is 25 of OD600 in a 10 mL system, and the initial concentration of styrene oxide is 4 g/L, then added 4 g/L every 4 h until it reached 20 g/L. The reaction was carried out in a 50 mL shaker at 30 °C, 200 rpm, and 100 µL aliquots of the mixture were taken out every 4 h before adding substrates. Then, centrifuged at 10,000 rpm for 1 min, 50 µL of supernatant was diluted with 950 µL ultrapure water and then filtered by 0.22 µm filter for HPLC analysis. R-MA was analyzed by HPLC equipped with an Aminex HPX-87H analysis column (Bio-Rad, 300 × 7.8 mm) and UV–Vis detector at 210 nm using 5 mM H2SO4 as eluent [69].

Membrane characteristics analysis

G. oxydans wild-type and G. oxydans STA cells were cultured to the same OD600 in log phase, then centrifuged and washed with PB buffer, and diluted to OD600 of 0.5. Propidium iodide (PI) was applied to analyze inner membrane permeability [70]. Taking 2 mL of dilutions into centrifuge tubes, 4 µL PI (1 g/L) were added and incubated in the dark for 5 min, harvested and washed twice. The controls were the same treatment using PB buffer replaced PI. The fluorescence intensity was measured under the excitation wavelength of 536 and emission wavelength of 617 using a fluorescence spectrophotometer. The inner membrane permeability was indicated by the absorption factor of PI and analyzed by the following formula: PI absorption factor = [F(PB + cells + PI)-F(PB + cells)]/[F(PB + PI)-F(PB)]. N-Phenyl-α-naphthylamine (NPN) was used to analyze the outer membrane permeability [71]. 200 µL sample dilutions were mixed with 2 µL NPN (10 mM), then the fluorescence intensity was detected by fluorescence spectrophotometer (excitation at 350 nm and emission at 420 nm).

The membrane integrity of G. oxydans strains were also analyzed using PI as the fluorescence dye, and the preparation of samples was the same as described above [72]. 500 µL dilutions with 3 µL PI were incubated in dark condition for 5 min, then measured by FACSCalibur flow cytometer with a rate of 500 to 800 cells/s and detected more than 20,000 cells. CellQuest software was used to collected and analyzed the results.

Membrane hydrophobicity of G. oxydans wild-type and G. oxydans STA cells were monitored by measuring the microbial adhesion to hydrocarbons (MATH) [46, 73]. After being collected and washed twice, the cells were suspended in PB buffer with a certain optical density at 550 nm (A0). 2.4 mL cell suspension together with 0.8 mL dodecane were vortexed at 1500 rpm for 10 min, then held for another 10 min to allow phase separation. Removed the organic layer and measured the absorbance (OD550) of the aqueous phase (A1). We used the following formula to calculate the percentage of cells into dodecane: (adhesion, %) = (A0–A1)/A0*100%. The adhesion was used as an indicator of the membrane hydrophobicity [74, 75].

Availability of data and materials

All data generated or analyzed during this study are included in this published article and its additional files.

References

  1. Rui L, Cao L, Chen W, Reardon KF, Wood TK. Protein engineering of epoxide hydrolase from Agrobacterium radiobacter AD1 for enhanced activity and enantioselective production of (R)-1-phenylethane-1,2-diol. Appl Environ Microbiol. 2005;71:3995.

    Article  CAS  Google Scholar 

  2. Zhu Y, Wang Q, Cornwall RG, Shi Y. Organocatalytic asymmetric epoxidation and aziridination of olefins and their synthetic applications. Chem Rev. 2014;114:8199–256.

    Article  CAS  Google Scholar 

  3. Panke S, Wubbolts MG, Schmid A, Witholt B. Production of enantiopure styrene oxide by recombinant Escherichia coli synthesizing a two-component styrene monooxygenase. Biotechnol Bioeng. 2015;69:91–100.

    Article  Google Scholar 

  4. Lukito BR, Sekar BS, Wu S, Li Z. Whole cell-based cascade biotransformation for the production of (S)-mandelic acid from styrene, L-phenylalanine, glucose, or glycerol. Adv Synth Catal. 2019;361:1–10.

    Article  Google Scholar 

  5. Liu S, Zhang X, Liu F, Xu M, Yang T, Long M, Zhou J, Osire T, Yang S, Rao Z. Designing of a cofactor self-sufficient whole-cell biocatalyst system for production of 1,2-amino alcohols from epoxides. ACS Synth Biol. 2019;8:734–43.

    Article  CAS  Google Scholar 

  6. Martínková L, Křen V. Biocatalytic production of mandelic acid and analogues: a review and comparison with chemical processes. Appl Microbiol Biotechnol. 2018;102:3893–900.

    Article  Google Scholar 

  7. Chang TL, Teleshova N, Rapista A, Paluch M, Anderson RA, Waller DP, Zaneveld LJD, Granelli-Piperno A, Klotman ME. SAMMA, a mandelic acid condensation polymer, inhibits dendritic cell-mediated HIV transmission. FEBS Lett. 2007;581:4596–602.

    Article  CAS  Google Scholar 

  8. Saravanan P, Singh VK. An efficient synthesis of chiral nonracemic diamines: application in asymmetric synthesis. Tetrahedron Lett. 1998;39:167–70.

    Article  CAS  Google Scholar 

  9. Chen X, Yang C, Wang P, Zhang X, Bao B, Li D, Shi R. Stereoselective biotransformation of racemic mandelic acid using immobilized laccase and (S)-mandelate dehydrogenase. Bioresour Bioprocess. 2017;4:2.

    Article  Google Scholar 

  10. Surivet J-P, Vatèle J-M. Total synthesis of antitumor Goniothalamus styryllactones. Tetrahedron. 1999;55:13011–28.

    Article  CAS  Google Scholar 

  11. Robinson CJ, Carbonell P, Jervis AJ, Yan C, Hollywood KA, Dunstan MS, Currin A, Swainston N, Spiess R, Taylor S, et al. Rapid prototyping of microbial production strains for the biomanufacture of potential materials monomers. Metab Eng. 2020;60:168–82.

    Article  CAS  Google Scholar 

  12. Yutthalekha T, Wattanakit C, Lapeyre V, Nokbin S, Warakulwit C, Limtrakul J, Kuhn A. Asymmetric synthesis using chiral-encoded metal. Nat Commun. 2016;7:12678.

    Article  CAS  Google Scholar 

  13. Zhao J, Liu Y, Hao A, Xing P. High-throughput synthesis of chiroptical nanostructures from synergistic hydrogen-bonded coassemblies. ACS Nano. 2020;14:2522–32.

    Article  CAS  Google Scholar 

  14. Lukito BR, Wang Z, Sekar BS, Li Z. Production of ( R )-mandelic acid from styrene, L-phenylalanine, glycerol, or glucose via cascade biotransformations. Bioresour Bioprocess. 2021;8:22.

    Article  Google Scholar 

  15. Reifenrath M, Boles E. Engineering of hydroxymandelate synthases and the aromatic amino acid pathway enables de novo biosynthesis of mandelic and 4-hydroxymandelic acid with Saccharomyces cerevisiae. Metab Eng. 2018;45:246–54.

    Article  CAS  Google Scholar 

  16. Wu S, Zhou Y, Wang T, Too H-P, Wang DIC, Li Z. Highly regio- and enantioselective multiple oxy- and amino-functionalizations of alkenes by modular cascade biocatalysis. Nat Commun. 2016;7:11917.

    Article  CAS  Google Scholar 

  17. Gao L, Hu Y, Liu J, Du G, Zhou J, Chen J. Stepwise metabolic engineering of Gluconobacter oxydans WSH-003 for the direct production of 2-keto-l-gulonic acid from d-sorbitol. Metab Eng. 2014;24:30–7.

    Article  CAS  Google Scholar 

  18. Zhou P, Yao R, Zhang H, Bao J. Unique glucose oxidation catalysis of Gluconobacter oxydans constitutes an efficient cellulosic gluconic acid fermentation free of inhibitory compounds disturbance. Biotechnol Bioeng. 2019;116:2191–9.

    Article  CAS  Google Scholar 

  19. Li D-H, Lin J-P, Wei D-Z. Improving Gluconobacter oxydans performance in the in situ removal of the inhibitor for asymmetric resolution of racemic 1-phenyl-1,2-ethanediol. Bioresour Technol. 2014;159:327–33.

    Article  CAS  Google Scholar 

  20. Wei L, Yang X, Gao K, Lin J, Yang S, Hua Q, Wei D. Characterization of Enzymes in the Oxidation of 1,2-Propanediol to D-(-)-Lactic Acid by Gluconobacter oxydans DSM 2003. Mol Biotechnol. 2010;46:26–33.

    Article  CAS  Google Scholar 

  21. Chao G, Wen Z, Huang Y, Ma C, Ping X. Efficient conversion of 1,2-butanediol to (R)-2-hydroxybutyric acid using whole cells of Gluconobacter oxydans. Bioresour Technol. 2012;115:75–8.

    Article  Google Scholar 

  22. Hua X, Du G, Zhou X, Nawaz A. A techno-practical method for overcoming the biotoxicity and volatility obstacles of butanol and butyric acid during whole-cell catalysis by Gluconobacter oxydans. Biotechnol Biofuels. 2020;13:102.

    Article  CAS  Google Scholar 

  23. Li G, Shan X, Zeng W, Yu S, Zhang G, Chen J, Zhou J. Efficient Production of 2,5-Diketo-D-gluconic Acid by Reducing Browning Levels During Gluconobacter oxydans ATCC 9937 Fermentation. Front Bioeng Biotechnol. 2022;10: 918277.

    Article  Google Scholar 

  24. Zou X, Lin J, Mao X, Zhao S, Ren Y. Biosynthesis of L-Erythrose by assembly of two key enzymes in Gluconobacter oxydans. J Agric Food Chem. 2017;65:7721–5.

    Article  CAS  Google Scholar 

  25. Matsushita K, Toyama H, Adachi O. Respiratory chains and bioenergetics of acetic acid bacteria. Adv Microb Physiol. 1994;36:247–301.

    Article  CAS  Google Scholar 

  26. Espinosa MI, Gonzalez-Garcia RA, Valgepea K, Plan MR, Scott C, Pretorius IS, Marcellin E, Paulsen IT, Williams TC. Adaptive laboratory evolution of native methanol assimilation in Saccharomyces cerevisiae. Nat Commun. 2020;11:5564.

    Article  CAS  Google Scholar 

  27. Ali F, Seshasayee ASN. Dynamics of genetic variation in transcription factors and its implications for the evolution of regulatory networks in Bacteria. Nucleic Acids Res. 2020;48:4100–14.

    Article  CAS  Google Scholar 

  28. Mohamed ET, Werner AZ, Salvachúa D, Singer CA, Szostkiewicz K, Rafael Jiménez-Díaz M, Eng T, Radi MS, Simmons BA, Mukhopadhyay A, et al. Adaptive laboratory evolution of Pseudomonas putida KT2440 improves p-coumaric and ferulic acid catabolism and tolerance. Metab Eng Commun. 2020;11: e00143.

    Article  Google Scholar 

  29. Wu Y, Jameel A, Xing X-H, Zhang C. Advanced strategies and tools to facilitate and streamline microbial adaptive laboratory evolution. Trends biotechnol. 2022;40:38–59.

    Article  Google Scholar 

  30. Zhu C, You X, Wu T, Li W, Chen H, Cha Y, Zhuo M, Chen B, Li S. Efficient utilization of carbon to produce aromatic valencene in Saccharomyces cerevisiae using mannitol as the substrate. Green Chem. 2022;24:4614.

    Article  CAS  Google Scholar 

  31. Zhou L, Xu Z, Wen Z, Lu M, Wang Z, Zhang Y, Zhou H, Jin M. Combined adaptive evolution and transcriptomic profiles reveal aromatic aldehydes tolerance mechanisms in Yarrowia lipolytica. Bioresource Technol. 2021;329: 124910.

    Article  CAS  Google Scholar 

  32. Caspeta L, Chen Y, Ghiaci P, Feizi A, Buskov S, Hallström BM, Petranovic D, Nielsen J. Biofuels. Altered sterol composition renders yeast thermotolerant. Science. 2014;346:75–8.

    Article  CAS  Google Scholar 

  33. Jin C, Hou W, Yao R, Zhou P, Zhang H, Bao J. Adaptive evolution of Gluconobacter oxydans accelerates the conversion rate of non-glucose sugars derived from lignocellulose biomass. Bioresource Technol. 2019;289:121623–121623.

    Article  CAS  Google Scholar 

  34. Wu S, Li A, Chin YS, Li Z. Enantioselective Hydrolysis of Racemic and Meso-Epoxides with Recombinant Escherichia coli Expressing Epoxide Hydrolase from Sphingomonas sp. HXN-200: Preparation of Epoxides and Vicinal Diols in High ee and High Concentration. ACS Catal. 2013;3:752–9.

    Article  CAS  Google Scholar 

  35. Cheng J-T, Yu J-H, Sun C-F, Cao F, Ying Y-M, Zhan Z-J, Li W-J, Chen X-A, Zhao Q-W, Li Y-Q, et al. A Cell Factory of a Fungicolous Fungus Calcarisporiumarbuscula for efficient production of natural products. ACS Synth Biol. 2021;10:698–706.

    Article  CAS  Google Scholar 

  36. Ruegg TL, Pereira JH, Chen JC, DeGiovanni A, Novichkov P, Mutalik VK, Tomaleri GP, Singer SW, Hillson NJ, Simmons BA, et al. Jungle Express is a versatile repressor system for tight transcriptional control. Nat Commun. 2018;9:3617.

    Article  Google Scholar 

  37. Ding N, Yuan Z, Zhang X, Chen J, Zhou S, Deng Y. Programmable cross-ribosome-binding sites to fine-tune the dynamic range of transcription factor-based biosensor. Nucleic Acids Res. 2020;89:10602–13.

    Article  Google Scholar 

  38. Boer CG, Vaishnav ED, Sadeh R, Abeyta EL, Friedman N, Regev A. Deciphering eukaryotic gene-regulatory logic with 100 million random promoters. Nat Biotechnol. 2020;38:56–65.

    Article  Google Scholar 

  39. Wilson EH, Groom JD, Sarfatis MC, Ford SM, Lidstrom ME, Beck DAC. A computational framework for identifying promoter sequences in nonmodel organisms using RNA-seq Data Sets. ACS Synth Biol. 2021;10:1394–405.

    Article  CAS  Google Scholar 

  40. Chen Y, Liu L, Yu S, Li J, Zhou J, Chen J. Identification of Gradient Promoters of Gluconobacter oxydans and Their Applications in the Biosynthesis of 2-Keto-L-Gulonic Acid. Front Bioeng Biotechnol. 2021;9: 673844.

    Article  Google Scholar 

  41. Li K, Mao X, Liu L, Lin J, Sun M, Wei D, Yang S. Overexpression of membrane-bound gluconate-2-dehydrogenase to enhance the production of 2-keto-D-gluconic acid by Gluconobacter oxydans. Microb Cell Fact. 2016;15:121.

    Article  Google Scholar 

  42. Yuan J, Wu M, Lin J, Yang L. Combinatorial metabolic engineering of industrial Gluconobacter oxydans DSM2343 for boosting 5-keto-D-gluconic acid accumulation. BMC Biotechnol. 2016;16:42.

    Article  Google Scholar 

  43. Pullmann P, Weissenborn MJ. Improving the heterologous production of fungal peroxygenases through an episomal Pichia pastoris promoter and signal peptide shuffling system. ACS Synth Biol. 2020;10:1360–72.

    Article  Google Scholar 

  44. Nora LC, Wehrs M, Kim J, Cheng JF, Tarver A, Simmons BA, Magnuson J, Harmon-Smith M, Silva-Rocha R, Gladden JM, et al. A toolset of constitutive promoters for metabolic engineering of Rhodosporidium toruloides. Microb Cell Fact. 2019;18:117.

    Article  Google Scholar 

  45. Pereira R, Wei Y, Mohamed E, Radi M, Malina C, Herrgård MJ, Feist AM, Nielsen J, Chen Y. Adaptive laboratory evolution of tolerance to dicarboxylic acids in Saccharomyces cerevisiae. Metab Eng. 2019;56:130–41.

    Article  CAS  Google Scholar 

  46. Santoscoy MC, Jarboe LR. A systematic framework for using membrane metrics for strain engineering. Metab Eng. 2021;66:98–113.

    Article  CAS  Google Scholar 

  47. Zhou P, Yuan X, Liu H, Qi Y, Chen X, Liu L. Candida glabrata Yap6 Recruits Med2 To Alter Glycerophospholipid Composition and Develop Acid pH Stress Resistance. Appl Environ Microb. 2020;86: e01915.

    Article  CAS  Google Scholar 

  48. Shin J, Yu J, Park M, Kim C, Kim H, Park Y, Ban C, Seydametova E, Song Y-H, Shin C-S, et al. Endocytosing Escherichia coli as a whole-cell biocatalyst of fatty acids. Acs Synth Biol. 2019;8:1055–66.

    Article  CAS  Google Scholar 

  49. Royce LA, Yoon JM, Chen Y, Rickenbach E, Shanks JV, Jarboe LR. Evolution for exogenous octanoic acid tolerance improves carboxylic acid production and membrane integrity. Metab Eng. 2015;29:180–8.

    Article  CAS  Google Scholar 

  50. Tan Z, Black W, Yoon JM, Shanks JV, Jarboe LR. Improving Escherichia coli membrane integrity and fatty acid production by expression tuning of FadL and OmpF. Microb Cell Fact. 2017;16:38.

    Article  Google Scholar 

  51. Lahesaare A, Ainelo H, Teppo A, Kivisaar M, Heipieper HJ, Teras R. LapF and its regulation by Fis affect the cell surface hydrophobicity of Pseudomonas putida. PLoS ONE. 2016;3: e0166078.

    Article  Google Scholar 

  52. Chen X, Song D, Xu J, Li E, Sun G, Xu M. Role and mechanism of cell-surface hydrophobicity in the adaptation of Sphingobium hydrophobicum to electronic-waste contaminated sediment. Appl Microbiol Biot. 2018;102:2803–15.

    Article  CAS  Google Scholar 

  53. Lim HG, Fong B, Alarcon G, Magurudeniya HD, Eng T, Szubin R, Olson CA, Palsson BO, Gladden JM, Simmons BA, et al. Generation of ionic liquid tolerant Pseudomonas putida KT2440 strains via adaptive laboratory evolution. Green Chem. 2020;22:5677.

    Article  CAS  Google Scholar 

  54. Pan X, Tang M, You J, Osire T, Sun C, Fu W, Yi G, Yang T, Yang S-T, Rao Z. PsrA is a novel regulator contributes to antibiotic synthesis, bacterial virulence, cell motility and extracellular polysaccharides production in Serratia marcescens. Nucleic Acids Res. 2022;50:127–48.

    Article  CAS  Google Scholar 

  55. Warrier T, Kapilashrami K, Argyrou A, Ioerger TR, Little D, Murphy KC, Nandakumar M, Park S, Gold B, Mi J, et al. N-methylation of a bactericidal compound as a resistance mechanism in Mycobacterium tuberculosis. Proc Natl Acad Sci U S A. 2016;113:E4523-4530.

    Article  CAS  Google Scholar 

  56. Gupta A, Pande A, Sabrin A, Thapa SS, Gioe BW, Grove A. MarR family transcription factors from Burkholderia species: hidden clues to control of virulence-associated genes. Microbiol Mol Biol R. 2018;83:e00039-e118.

    Google Scholar 

  57. Huang Y, Suo Y, Shi C, Szlavik J, Shi X-M, Knøchel S. Mutations in gltB and gltC reduce oxidative stress tolerance and biofilm formation in Listeria monocytogenes 4b G. Int J Food Microbiol. 2013;163:223–30.

    Article  CAS  Google Scholar 

  58. Martin RG, Rosner JL. The AraC transcriptional activators. Curr Opin Microbiol. 2001;4:132–7.

    Article  CAS  Google Scholar 

  59. Tobes R, Ramos JL. AraC-XylS database: a family of positive transcriptional regulators in bacteria. Nucleic Acids Res. 2002;30:318–21.

    Article  CAS  Google Scholar 

  60. Nishino K, Senda Y, Hayashi-Nishino M, Yamaguchi A. Role of the AraC-XyIS family regulator YdeO in multi-drug resistance of Escherichia coli. J Antibiot. 2009;62:251–7.

    Article  CAS  Google Scholar 

  61. Barraud N, Létoffé S, Beloin C, Vinh J, Chiappetta G, Ghigo J-M. Lifestyle-specific S-nitrosylation of protein cysteine thiols regulates Escherichia coli biofilm formation and resistance to oxidative stress. Biofilms Microbi. 2020;7:34.

    Article  Google Scholar 

  62. Mikolosko J, Bobyk K, Zgurskaya HI, Ghosh P. Conformational flexibility in the multidrug efflux system protein AcrA. Structure. 2006;14:577–87.

    Article  CAS  Google Scholar 

  63. Nikaido H. Multidrug resistance in bacteria. Annu Rev Biochem. 2009;78:119–46.

    Article  CAS  Google Scholar 

  64. Li X-Z, Plésiat P, Nikaidoc H. The challenge of efflux-mediated antibiotic resistance in gram-negative bacteria. Clin Microbiol Rev. 2015;28:337–418.

    Article  Google Scholar 

  65. Alav I, Kobylka J, Kuth MS, Pos KM, Picard M, Blair JMA, Bavro VN. Structure, assembly, and function of tripartite efflux and type 1 secretion systems in gram-negative bacteria. Chem Rev. 2021;121:5479–596.

    Article  CAS  Google Scholar 

  66. Plé C, Tam H-K, Cruz AVD, Compagne N, Jiménez-Castellanos J-C, Müller RT, Pradel E, Foong WE, Malloci G, Ballée A, et al. Pyridylpiperazine-based allosteric inhibitors of RND-type multidrug efflux pumps. Nat Commun. 2022;13:115.

    Article  Google Scholar 

  67. Kusumawardhani H, Furtwängler B, Blommestijn M, Kaltenytė A. Adaptive laboratory evolution restores solvent tolerance in plasmid-cured Pseudomonas putida S12: a molecular analysis. Appl Environ Microb. 2021;87:e00041-e121.

    Article  CAS  Google Scholar 

  68. Prust C, Hoffmeister M, Liesegang H, Wiezer A, Fricke WF, Ehrenreich A, Gottschalk G, Deppenmeier U. Complete genome sequence of the acetic acid bacterium Gluconobacter oxydans. Nat Biotechnol. 2005;23:195.

    Article  CAS  Google Scholar 

  69. Zhou J, Zhang R, Yang T, Liu Q, Zheng J, Wang F, Liu F, Xu M, Zhang X, Rao Z. Relieving Allosteric Inhibition by Designing Active Inclusion Bodies and Coating of the Inclusion Bodies with Fe3O4 Nanomaterials for Sustainable 2-Oxobutyric Acid Production. ACS Catal. 2018;8:8889–901.

    Article  CAS  Google Scholar 

  70. Yao C, Rudnitzki F, Hüttmann G, Zhang Z, Rahmanzadeh R. Important factors for cell-membrane permeabilization by gold nanoparticles activated by nanosecond-laser irradiation. Int J Nanomed. 2017;12:5659–72.

    Article  CAS  Google Scholar 

  71. Loh B, Grant C, Hancock REW. Use of the fluorescent probe 1-N-phenylnaphthylamine to study the interactions of aminoglycoside antibiotics with the outer membrane of Pseudomonas aeruginosa. Antimicrob Agents Ch. 1984;26:546–51.

    Article  CAS  Google Scholar 

  72. Baars L, Wagner S, Wickström D, Klepsch M, Ytterberg AJ. Effects of SecE Depletion on the Inner and Outer Membrane Proteomes of Escherichia coli. J Bacteriol. 2008;190:24–24.

    Article  Google Scholar 

  73. Loosdrecht MCMV, Lyklema J, Norde W, Schraa G, Zehnder AJB. The role of bacterial cell wall hydrophobicity in adhesion. Appl Environ Microbiol. 1987;53:1893–7.

    Article  Google Scholar 

  74. Rosenberg M, Gutnick D, Rosenberg E. Adherence of bacteria to hydrocarbons: a simple method for measuring cell-surface hydrophobicity. FEMS Microbiol Lett. 1980;9:29–33.

    Article  CAS  Google Scholar 

  75. Hamadi F, Latrache H. Comparison of contact angle measurement and microbial adhesion to solvents for assaying electron donor-electron acceptor (acid-base) properties of bacterial surface. Colloids Surf B Biointerfaces. 2008;65:134–9.

    Article  CAS  Google Scholar 

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Funding

This work was supported by the National Key Research and Development Program of China, (No. 2021YFC2100900), National Natural Science Foundation of China (Nos. 32171471, 32071470), the Project Funded by the Priority Academic Program Development of Jiangsu Higher Education Institutions and Top-notch Academic Programs Project of Jiangsu Higher Education Institutions.

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FL wrote the manuscript draft; FL, JPZ and MKH performed the major experiments. YC and JH analyzed the data. XWP and JJY revised the manuscript; MJX, TWY and MLS edited the manuscript; XZ and ZMR designed the research. All authors read and approved the final manuscript.

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Additional file 1:

Fig. S1 (a) SDS–PAGE of SpEH expression strains. Lane M: protein marker; Lane 1: whole cell protein of wild-type G. oxydans without overexpressing SpEH; Lane 2: whole cell protein of WT-SpEH; Lane 3: whole cell protein of G. oxydans STA without overexpressing SpEH; Lane 4: whole cell protein of STA-SpEH. (b) Enzyme activity of crude SpEH of WT-SpEH and STA-SpEH. Fig. S2. Membrane permeability and hydrophobicity analysis of G. oxydans STA strains. (a) NPN fluorescence intensity analyses of outer membrane permeability in STA stains. (b) Inner membrane permeability change of propidium iodide (PI) uptake factor in STA stains. (c) Membrane hydrophobicity was changed STA stains. **P < 0.01. ***P < 0.001. Table S1. Strains used in this study. Table S2. Primers used in this study. Table S3. Gene IDs and protein functions of promoters.

Additional file 2: Table S4.

1. Comparative genomic analysis of WT VS STA. 2. Key mutations in the evolved strain STA. 3. Differentially expressed gene of WT VS WT-3g. 4. Differentially expressed gene of STA VS STA-3g. 5. Differentially expressed gene of WT VS STA. 6. Differentially expressed gene of WT-3g VS STA-3g.

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Liu, F., Zhou, J., Hu, M. et al. Efficient biosynthesis of (R)-mandelic acid from styrene oxide by an adaptive evolutionary Gluconobacter oxydans STA. Biotechnol Biofuels 16, 8 (2023). https://doi.org/10.1186/s13068-023-02258-7

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  • Accepted:

  • Published:

  • DOI: https://doi.org/10.1186/s13068-023-02258-7

Keywords

  • (R)-mandelic acid
  • Gluconobacter oxydans
  • Adaptive laboratory evolution
  • Promoters
  • Styrene oxide
  • Biotransformation