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Efficient 1,3-dihydroxyacetone biosynthesis in Gluconobacter oxydans using metabolic engineering and a fed-batch strategy
Bioresources and Bioprocessing volume 9, Article number: 121 (2022)
1,3-Dihydroxyacetone (DHA) is a commercially important chemical and widely used in cosmetics, pharmaceuticals, and food industries as it prevents excessive water evaporation, and provides anti-ultraviolet radiation protection and antioxidant activity. Currently, the industrial production of DHA is based on a biotechnological synthetic route using Gluconobacter oxydans. However, achieving higher production requires more improvements in the synthetic process. In this study, we compared DHA synthesis levels in five industrial wild-type Gluconobacter strains, after which the G. oxydans WSH-003 strain was selected. Then, 16 dehydrogenase genes, unrelated to DHA synthesis, were individually knocked out, with one strain significantly enhancing DHA production, reaching 89.49 g L−1 and 42.27% higher than the wild-type strain. By optimizing the culture media, including seed culture and fermentation media, DHA production was further enhanced. Finally, using an established fed-batch fermentation system, DHA production reached 198.81 g L−1 in a 5 L bioreactor, with a glycerol conversion rate of 82.84%.
1,3-Dihydroxyacetone (DHA) is a commercially important chemical and is widely used in cosmetics, pharmaceutical, and food industries (Dikshit et al. 2017; Turner et al. 2022). DHA reacts with amino acids in the skin cuticle to generate a brown protective film to prevent excessive water evaporation, promote moisturization, and provide sun and anti-ultraviolet radiation protection. DHA does not cause any harmful effects to the skin, as it has been a common active ingredient in sunless tanning skincare preparations (Jankowski et al. 2016; Perer et al. 2020; Perrin, 2020). Due to its ability to turn the skin brown, DHA is also used as a treatment or adjunctive treatment for some skin diseases, such as white spot, psoriasis, and vitiligo (Li et al. 2021b). It was also proposed as a food additive, while DHA effectively promoted body fat reduction and increased endurance (Obeid et al. 2006). In addition, DHA is an essential precursor for the production of different fine chemicals, and serves as a building block for the synthesis of new non-toxic and biodegradable polymers (Dikshit et al. 2018; Korley et al. 2016).
The industrial production of DHA mainly relies on chemical synthesis and biotechnological synthetic routes (Dikshit & Moholkar, 2016a; Tateno et al. 2022). The chemical synthesis method includes formaldehyde condensation and glycerol oxidation; however, the method is problematic as it is difficult to strike a balance between synthesis conditions and material costs. In addition, the method is disadvantageous in terms of low product purity, over oxidation levels, and high costs which limit DHA production (de la Morena et al. 2019). The biotechnological synthetic route is superior in terms of mild reaction conditions, strong specificity, high substrate utilization, a simple process, and therefore, this route has become the main DHA production industrial method (Dobson et al. 2012; Ripoll et al. 2021). Several microorganisms accumulate DHA using glycerol as a substrate, including Acetobacter, Gluconobacter, Klebsiella, and Pichia, of which Gluconobacter oxydans is generally considered the most desirable and widely used DHA producer (Ko et al. 2020; Lin et al. 2016; Liu et al. 2008).
G. oxydans is a classical obligate aerobic bacterium and has a complicated and powerful dehydrogenase system, with an unmatched capacity to effectively and efficiently oxidize alcohols, carbohydrates, and related compounds (Qin et al. 2022). Based on these properties, the organisms is widely used for the industrial production of D-gluconic acid, miglitol, vitamin C, and DHA (da Silva et al. 2022; Li et al. 2022; Ripoll et al. 2021). DHA accumulation commonly relies on a membrane-bound glycerol dehydrogenase (GLDH), which is a pyrroloquinoline quinone dependent enzyme. Studies have reported that GLDH has a wide substrate spectrum as many polyhydric alcohols can be oxidized, such as D-sorbitol, D-arabitol, D-mannitol, and adonitol (Dikshit et al. 2017; Lapenaite et al. 2005). To enhance DHA production, several strategies have been used, including generating high-producing strains using random mutagenesis and gene recombination, optimizing fermentation culture medium and control conditions, and establishing resting cells and immobilized processes (Dikshit et al. 2018; Hu & Zheng, 2011; Kataoka et al. 2021).
In this study, the G. oxydans WSH-003 strain, selected from five industrial wild-type Gluconobacter strains, generated the best DHA yields. To further enhance DHA production, 16 dehydrogenase genes, unrelated to DHA synthesis, were knocked out by metabolic engineering. We showed that 11 strains, which had 11 different and separate knocked out dehydrogenase genes, significantly promoted DHA production, of which G. oxydans WSH-003–4 accumulated a 42.27% higher DHA titer than the original G. oxydans WSH-003 strain. After optimizing seed culture and fermentation media compositions, the DHA production was further increased. Finally, using an intermittent fed-batch strategy, the DHA production was enhanced to 198.81 g L−1. Our data provide a reference point for enhancing the synthetic efficiency of target compounds in G. oxydans.
Materials and methods
Five wild-type Gluconobacter strains were used in this study: (1) G. oxydans WSH-004, (2) G. oxydans WSH-003, (3) G. oxydans 621H, (4) Gluconobacter japonicus CGMCC 1.49, and (5) Gluconobacter cerinus CGMCC 1.110 (Liu et al. 2021). Escherichia coli JM109 was used for plasmid construction. A list of study strains is shown in Table 1.
Medium and cultivation
The solid slant medium method was used for strain activation and comprised 40 g L−1 L-sorbitol, 10 g L−1 yeast extract powder, and 20 g L−1 agar. Initial seed medium comprised 50 g L−1 glucose and 10 g L−1 yeast extract powder, and corresponding initial fermentation medium consisted of 50 or 100 g L−1 glycerol and 10 g L−1 yeast extract powder. Improved seed medium comprised 60 g L−1 L-sorbitol and 20 g L−1 yeast extract powder, and corresponding improved fermentation medium comprised 50 or 100 g L−1 glycerol and 20 g L−1 yeast extract powder, 5 g L−1 CaCO3, 1 g L−1 MgSO4·7H2O, 0.9 g L−1 KH2PO4, and 0.13 g L−1 K2HPO4·3H2O (pH 6.2). The final optimized seed medium contained 60 g L−1 L-sorbitol and 10 g L−1 yeast extract powder, and the final optimized fermentation medium consisted of 100 g L−1 glycerol and 15 g L−1 yeast extract, 5 g L−1 CaCO3, 1 g L−1 MgSO4·7H2O, 0.9 g L−1 KH2PO4, and 0.13 g L−1 K2HPO4·3H2O (pH 6.2).
DHA strains were incubated on solid slant medium at 30 °C for 48 h. Seed culture and fermentation cultivation were initialized in 500 mL shaking flasks plus 50 mL fermentation seed medium at 30 °C and 200 rpm in a reciprocal shaker (Zhichu, Shanghai, China). Fermentation was performed in a 5 L bioreactor (T&J Bio-engineering, Shanghai, China) containing a 3 L working volume with an agitation speed of 600 rpm, a 2.0 vvm, and 30 °C. The all inoculation size was 6% (v/v).
Knocking out dehydrogenase genes and constructing engineered strains
Up- and down-stream homologous arms of 16 selected dehydrogenase genes were generated by polymerase chain reaction (PCR) from the G. oxydans WSH-003 genome (primer details are provided in Additional file 1). The kana gene was amplified from a pBBR-MCS-2 plasmid and individually fused to the up- and down-stream homologous arms of respective dehydrogenase genes. Sixteen fused fragments corresponding to dehydrogenase genes were generated. Then, 16 engineered strains were constructed by integrating the designed fused fragments into the G. oxydans WSH-003 parental strain to generate knock-out dehydrogenase gene strains (Liu et al. 2022a; Zeng et al. 2019).
Biomass determination: samples at different fermentation timepoints were diluted to an appropriate concentration with 1 M HCl. The optical density was determined at 600 nm.
Glycerol and DHA determination: glycerol and DHA concentrations in fermentation samples were detected using high-performance liquid chromatography (HPLC, Shimadzu, Kyoto, Japan) equipped with an Aminex HPX-87H column (Bio-Rad, CA, USA). HPLC detection conditions: 10 µL of injection volume, 5 mM H2SO4 of mobile phase with an elution rate of 0.5 mL·min−1, and column temperature of 40 °C. DHA was detected using a UV detector at 271 nm and glycerol detected using a refractive index detector.
The experimental data were analyzed by Origin 2019b, and the significant differences were analyzed using student’s T tests.
Results and discussion
Screening strains for optimal DHA production
For improved DHA production, different Gluconobacter sp. strains have been studied and included Gluconobacter frateurii, Gluconobacter thailandicus, and G. oxydans (de la Morena et al. 2020; Jittjang et al. 2020; Poljungreed & Boonyarattanakalin, 2017). To identify optimal DHA production, five wild-type industrial strains, G. oxydans WSH-004, G. oxydans WSH-003, G. oxydans 621H, G. japonicus CGMCC 1.49, and G. cerinus CGMCC 1.110 were selected and compared (Liu et al. 2021). After well activating, strains were grown in fermentation media containing 50 g L−1 and 100 g L−1 glycerol as initial substrates. DHA titers in G. oxydans WSH-003 and G. cerinus CGMCC 1.110 fermentations were higher than the other strains, but when glycerol levels increased to 100 g L−1, DHA production decreased (Fig. 1A).
To solve this issue and identify the best DHA producer from G. oxydans WSH-003 and G. cerinus CGMCC 1.110 strains, both were compared using an improved seed medium that L-sorbitol as carbon source replacing glucose, and the corresponding fermentation medium that adding some significant inorganic salts, such as MgSO4·7H2O and KH2PO4 (Dikshit & Moholkar, 2016b; Hu et al. 2010a). As indicated in Fig. 1B, the G. oxydans WSH-003 strain performed relatively better, accumulating 64.48 g L−1 DHA in 100 g L−1 initial glycerol, higher than G. cerinus CGMCC 1.110 (60.16 g L−1). In addition, in the improved culture medium, DHA accumulation with G. oxydans WSH-003 was greatly enhanced at 100 g L−1 initial glycerol and was higher than 50 g L−1 initial glycerol (38.84 g L−1). The conversion rate with 100 g L−1 initial glycerol (64.48%) was lower than that of with 50 g L−1 initial glycerol (77.68%), but the productivity with 100 g L−1 initial glycerol (0.90 g L−1 h−1) is obvious higher than that of with 50 g L−1 initial glycerol (0.54 g L−1 h−1). Considering the DHA concentration, conversion rate and productivity, addition of 100 g L−1 initial glycerol was selected.
Effects of knocking out dehydrogenase genes on DHA accumulation
Gluconobacter has a considerably complex but functional dehydrogenase system, whereby various alcohols/sugars/ketones are rapidly and incompletely oxidized to corresponding sugars/ketones/acids. However, this powerful dehydrogenase system appears to be disordered, such that specific substrates may be oxidized by different dehydrogenases, easily leading to formation of several by-products, which always could be rapidly converted to synthesis of other metabolites or biomass, thereby reducing target product titers (Liu et al. 2022a; Wang et al. 2018). Besides, the competitive dehydrogenases could reduce efficiency of coenzyme for synthesis of target products (Qin et al. 2022; Wang et al. 2016). To enhance the production of specific target compounds in Gluconobacter, metabolic engineering strategies involving knock-out or repressing unrelated dehydrogenase genes have been conducted (Liu et al. 2022a; Qin et al. 2021). In previous work, knocking out mgdh which encoded a membrane-bound glucose dehydrogenase and adh which encoded a membrane-bound alcohol dehydrogenase enhanced DHA titers (Lu et al. 2012). In addition, based on complete genome sequences, more dehydrogenase genes related to alcohols oxidization have been identified in Gluconobacter (Prust et al., 2005).
To investigate the effects of other dehydrogenase knockout strains on DHA accumulation, 16 identified dehydrogenase genes (the identified possible characteristic of these genes were presented in Additional file 1) unrelated to DHA synthesis were selected and individually knocked out. However, according to our experience, these annotated characteristics cannot fully reflect their real functions. In general, they can convert more substrates than the annotated names. The resulting strains were cultured in shaking flasks in a proven fermentation medium plus 100 g L−1 glycerol. The wild-type G. oxydans WSH-003 strain was used as a control. Results showed that knocking out of these dehydrogenase genes have no obvious effect on cell growth. All engineered strains promoted DHA accumulation; 11 strains induced significant effects, enhancing DHA production by 26.01%, 29.30%, 31.22%, 42.27%, 29.21%, 33.39%, 23.97%, 27.81%, 26.84%, 26.22%, and 23.43%, respectively (Fig. 2). The highest DHA titer (89.49 g L−1) was generated by G. oxydans WSH-003–4, where the alcohol dehydrogenase 4 was knocked out—productivity was 1.24 g L−1 h−1. In addition, same to the original strain G. oxydans WSH-003, no obvious by-product was detected in fermentation broth with the engineered strains. The specific mechanisms of influences of these dehydrogenases on DHA accumulation need to be further explored in the future. The fermentation characteristics of each engineered strain are shown in Table 2.
Optimizing culture media for DHA production
To optimize DHA production with G. oxydans WSH-003–4, we investigated the effects of reducing L-sorbitol and yeast extract powder, and replacing yeast extract powder with a cheaper yeast extract in seed culture medium. Appropriately decreased yeast extract powder levels of seed culture medium were more conducive to DHA synthesis, and a high 91.28 g L−1 DHA titer was harvested using a combination of 60 g L−1 L-sorbitol and 10 g L−1 yeast extract powder. However, further reducing the L-sorbitol concentration and replacing yeast extract powder with yeast extract decreased the DHA titer (Fig. 3A). After seed culture medium optimization, the addition of two cheaper nitrogen sources (yeast extract and corn steep liquor) to fermentation medium, and their effects on DHA production, were compared with original yeast extract powder. A relatively higher DHA titer was determined with yeast extract as the nitrogen source; 93.88 g L−1 and 93.94 g L−1 DHA were generated by 15 g L−1 and 20 g L−1, respectively. Finally, 15 g·L−1 yeast extract addition was selected after comprehensive comparison (Fig. 3B). Comparing the additions in seed culture medium and fermentation medium, it was indicated that a suitable type and concentration of nitrogen source was of significance, since nitrogen sources could affect growth rate of strain and further affect activity of strain.
To bacterially biosynthesize specific target products in a fermentation procedure, culture media, including seed culture and fermentation media are important factors (de la Morena et al. 2019; Wang et al. 2014). A suitable culture medium could improve the target product accumulation. For example, by optimizing seed culture medium composition, ansamitocin production by Actinosynnema was increased by 26.8% (Li et al. 2021a). By optimizing different inorganic salts and nitrogen sources in fermentation culture medium, DHA production by G. oxydans was promoted and the production period decreased (Dikshit & Moholkar, 2016b; Hu et al. 2010a). In our study, by optimizing seed culture medium composition with respect to L-sorbitol and yeast extract, and comparing different nitrogen sources in the fermentation medium, the DHA production was further enhanced.
Batch fermentation with different initial glycerol concentrations in a 5 L bioreactor
With improved seed and fermentation medium, the issue that DHA production decreased when glycerol concentration increased was well-solved, and DHA production further enhanced by optimizing the culture medium in shaking flasks. The effects of different initial glycerol concentrations (100 g L−1, 120 g L−1, and 140 g L−1) on DHA production by G. oxydans WSH-003–4 were further investigated in a 5 L bioreactor (Fig. 4). When compared with fermentation in shaking flasks, fermentation period in the bioreactor were significantly shortened. The highest DHA production level was identified at 120 g L−1 glycerol for 46 h, reaching 109.18 g L−1, with a conversion rate of 90.98% and a productivity of 2.37 g L−1 h−1, and better than 100 g L−1 initial glycerol (its highest DHA titer was 85.25 g L−1 for 42 h, with a conversion rate of 85.25% and productivity of 2.03 g L−1 h−1). When initial glycerol was increased to 140 g L−1, the highest DHA titer was just 96.56 g L−1, while the fermentation period was 60 h.
Glycerol is a renewable, sustainable, and carbon neutral resource, which is a by-product generated during biodiesel manufacturing processes (Liu et al. 2022b; Luo et al. 2016). It is directly used as a sole carbon source by microorganisms for cell growth and target product synthesis via oxidation and reduction pathways. As it is abundant, available, and easy to absorb, glycerol has become a principal industrial substrate for the production of diverse value-added compounds via biotechnological routes, including the production of erythritol, 1,3-propanediol, organic acids, polyhydroxyalkanoates, exopolysaccharide, biosurfactants, and DHA (Ripoll et al. 2021; Westbrook et al. 2019; Zhang et al. 2021). For DHA production in G. oxydans, it was previously shown that high glycerol concentrations inhibited DHA synthesis (Hu et al. 2010b). Similarly, we demonstrated that DHA production efficiency was reduced at 140 g L−1 initial glycerol. However, DHA inhibition could be relieved by adding low glycerol concentrations, but titers were also reduced. To ensure production efficiency, an appropriate initial glycerol concentration was necessary (Stasiak-Rozanska et al. 2014).
Enhanced DHA production using a fed-batch fermentation strategy
Based on batch fermentation data, fed-batch strategy was investigated to improve DHA production by G. oxydans WSH-003–4. Using an initial 120 g L−1 glycerol, 20 g L−1 was fed at 1 time when residual glycerol concentration was < 5 g L−1. The process, using an initial 100 g L−1 glycerol and feeding 40 g L−1 at 1 time, was as a control. The process that using an initial 120 g L−1 glycerol and feeding 20 g L−1 yielded a better results. 122.23 g L−1 DHA was obtained (Fig. 5B), while the control process produced 116.16 g L−1 DHA (Fig. 5A). To further enhance the production, an intermittent fed-batch fermentation strategy was proposed, that is using an initial 120 g L−1 glycerol, 20 g L−1 was fed once residual glycerol concentration was < 5 g L−1, and 6 times of feeding was conducted. 198.81 g L−1 DHA was generated (conversion rate = 82.84%, productivity = 1.84 g L−1 h−1) (Fig. 5C). Characteristics of different fermentation processes, based on 120 g L−1 initial glycerol, are shown in Table 3.
Fed-batch fermentation processes could enhance target product accumulation. This was particularly relevant to DHA as high glycerol concentrations inhibited DHA synthesis. Based on different producer and corresponding synthetic compound characteristics, diverse fed-batch fermentation strategies have been successfully developed and include a single-dose fed-batch fermentation for 2-phenylethanol production using Wickerhamomyces anomalus (Tian et al. 2020), a constant-rate feeding fermentation method for α-ketoglutaric acid production using Yarrowia lipolytica (Zeng et al. 2017), and an intermittent fed-batch fermentation method for 2-keto-D-gluconic acid using Gluconobacter japonicas (Zeng et al. 2019). In our study, higher DHA production levels were generated, but glycerol conversion rate and productivity were required to improve when compared with reported results (Hu et al. 2010a). In future studies, increased efforts must be made to combine fed-batch fermentation with dissolved oxygen or pH control measures. These two parameters are important factors for alcohol oxidation using Gluconobacter (Hanke et al. 2012; Poljungreed and Boonyarattanakalin, 2017).
To enhance DHA production, the G. oxydans WSH-003 strain was selected from five industrial wild-type strains. By knocking out individual dehydrogenase genes unrelated to DHA synthesis, a suite of engineered strains was constructed. The G. oxydans WSH-003–4 strain yielded 89.49 g L−1 DHA, enhancing production by 42.27%. By optimizing culture media in flasks, DHA production was further enhanced, while the addition of organic nitrogen source in culture media was decreased. Furthermore, using an intermittent fed-batch fermentation strategy, 198.81 g L−1 DHA was generated in a 5 L bioreactor, with a glycerol conversion rate of 82.84%. We provide a reference point for the industrial production of DHA and other chemicals using Gluconobacter.
Availability of data and materials
All data generated or analyzed during this study are included in this published article and its Additional files.
da Silva GAR, Oliveira SSD, Lima SF, Nascimento RP, Baptista ARD, Fiaux SB (2022) The industrial versatility of Gluconobacter oxydans: current applications and future perspectives. World J Microbiol Biot 38(8):134
de la Morena S, Acedos MG, Santos VE, Garcia-Ochoa F (2019) Dihydroxyacetone production from glycerol using Gluconobacter oxydans: study of medium composition and operational conditions in shaken flasks. Biotechnol Progr 35(4):e2803
de la Morena S, Wojtusik M, Santos VE, Garcia-Ochoa F (2020) Kinetic modeling of dihydroxyacetone production from glycerol by Gluconobacter oxydans ATCC 621 resting cells: effect of fluid dynamics conditions. Catalysts 10(1):101
Dikshit PK, Moholkar VS (2016a) Kinetic analysis of dihydroxyacetone production from crude glycerol by immobilized cells of Gluconobacter oxydans MTCC 904. Bioresource Technol 216:948–957
Dikshit PK, Moholkar VS (2016b) Optimization of 1,3-dihydroxyacetone production from crude glycerol by immobilized Gluconobacter oxydans MTCC 904. Bioresource Technol 216:1058–1065
Dikshit PK, Padhi SK, Moholkar VS (2017) Process optimization and analysis of product inhibition kinetics of crude glycerol fermentation for 1,3-dihydroxyacetone production. Bioresource Technol 244:362–370
Dikshit PK, Kharmawlong GJ, Moholkar VS (2018) Investigations in sonication-induced intensification of crude glycerol fermentation to dihydroxyacetone by free and immobilized Gluconobacter oxydans. Bioresource Technol 256:302–311
Dobson R, Gray V, Rumbold K (2012) Microbial utilization of crude glycerol for the production of value-added products. J Ind Microbiol Biot 39(2):217–226
Hanke T, Richhardt J, Polen T, Sahm H, Bringer S, Bott M (2012) Influence of oxygen limitation, absence of the cytochrome bc(1) complex and low pH on global gene expression in Gluconobacter oxydans 621H using DNA microarray technology. J Biotechnol 157(3):359–372
Hu ZC, Zheng YG (2011) Enhancement of 1,3-dihydroxyacetone production by a UV-induced mutant of Gluconobacter oxydans with DO control strategy. Appl Biochem Biotech 165(5–6):1152–1160
Hu ZC, Liu ZQ, Zheng YG, Shen YC (2010a) Production of 1,3-dihydroxyacetone from glycerol by Gluconobacter oxydans ZJB09112. J Microbiol Biotechn 20(2):340–345
Hu ZC, Zheng YG, Shen YC (2010b) Dissolved-oxygen-stat fed-batch fermentation of 1,3-dihydroxyacetone from glycerol by Gluconobacter oxydans ZJB09112. Biotechnol Bioproc Eng 15(4):651–656
Jankowski M, Nowowiejska L, Czajkowski R (2016) Wood’s lamp fluorescence of dihydroxyacetone treated skin. J Eur Acad Dermatolo 30(11):E125–E126
Jittjang S, Jiratthiticheep I, Kajonpradabkul P, Tiatongjitman T, Siriwatwechakul W, Boonyarattanakalin S (2020) Effect of NaCl removal from biodiesel-derived crude glycerol by ion exchange to enhance dihydroxyacetone production by Gluconobacter thailandicus in minimal medium. J Chem Technol Biot 95(1):281–288
Kataoka N, Hirata K, Matsutani M, Ano Y, Nguyen TM, Adachi O, Matsushita K, Yakushi T (2021) Three ATP-dependent phosphorylating enzymes in the first committed step of dihydroxyacetone metabolism in Gluconobacter thailandicus NBRC3255. Appl Microbiol Biotechnol 105(3):1227–1236
Ko GS, Nguyen QT, Kim DH, Yang JK (2020) Biochemical and molecular characterization of glycerol dehydrogenase from Klebsiella pneumoniae. J Microbiol Biotechn 30(2):271–278
Korley JN, Yazdi S, McHugh K, Kirk J, Anderson J, Putnam D (2016) One-step synthesis, biodegradation and biocompatibility of polyesters based on the metabolic synthon, dihydroxyacetone. Biomaterials 98:41–52
Lapenaite I, Kurtinaitiene B, Razumiene J, Laurinavicius V, Marcinkeviciene L, Bachmatova I, Meskys R, Ramanavicius A (2005) Properties and analytical application of PQQ-dependent glycerol dehydrogenase from Gluconobacter sp 33. Anal Chim Acta 549(1–2):140–150
Li J, Guo SY, Hua Q, Hu FX (2021a) Improved AP-3 production through combined ARTP mutagenesis, fermentation optimization, and subsequent genome shuffling. Biotechnol Lett 43(6):1143–1154
Li M, Wang F, Ding XL, Xu QX, Du J (2021b) Evaluation of the potential interference of camouflage on the treatment of vitiligo: an observer-blinded self-controlled study. Dermatol Ther 34(1):e14545
Li D, Liu L, Qin ZJ, Yu SQ, Zhou JW (2022) Combined evolutionary and metabolic engineering improve 2-keto-L-gulonic acid production in Gluconobacter oxydans WSH-004. Bioresource Technol 354:127107
Lin X, Liu S, Xie GR, Chen J, Li PH, Chen JH (2016) Enhancement of 1,3-dihydroxyacetone production from Gluconobacter oxydans by combined mutagenesis. J Microbiol Biotechol 26(11):1908–1917
Liu ZQ, Hu ZC, Zheng YG, Shen YC (2008) Optimization of cultivation conditions for the production of 1,3-dihydroxyacetone by Pichia membranifaciens using response surface methodology. Biochem Eng J 38(3):285–291
Liu L, Chen Y, Yu SQ, Chen J, Zhou JW (2021) Simultaneous transformation of five vectors in Gluconobacter oxydans. Plasmid 117:102588
Liu L, Chen Y, Yu SQ, Chen J, Zhou JW (2022a) Enhanced production of L-sorbose by systematic engineering of dehydrogenases in Gluconobacter oxydans. Synth Syst Biotechnol 7(2):730–737
Liu Y, Wang M, Zhang B, Yan DP, Xiang X (2022b) Mediating the oxidizing capability of surface-bound hydroxyl radicals produced by photoelectrochemical water oxidation to convert glycerol into dihydroxyacetone. ACS Catal 12(12):6946–6957
Lu LF, Wei LJ, Zhu K, Wei DZ, Hua Q (2012) Combining metabolic engineering and adaptive evolution to enhance the production of dihydroxyacetone from glycerol by Gluconobacter oxydans in a low-cost way. Bioresource Technol 117:317–324
Luo XL, Ge XM, Cui SQ, Li YB (2016) Value-added processing of crude glycerol into chemicals and polymers. Bioresource Technol 215:144–154
Obeid OA, Jamal ZM, Hwalla N, Emery PW (2006) The effect of glutamine and dihydroxyacetone supplementation on food intake, weight gain, and postprandial glycogen synthesis in female Zucker rats. Nutrition 22(7–8):794–801
Perer J, Jandova J, Fimbres J, Jennings EQ, Galligan JJ, Hua A, Wondrak GT (2020) The sunless tanning agent dihydroxyacetone induces stress response gene expression and signaling in cultured human keratinocytes and reconstructed epidermis. Redox Biol 36:101594
Perrin DM (2020) A hypothesis for examining dihydroxyacetone, the active component in sunless tanning products, as a topical prophylactic against SARS-COV-2 transmission. Med Hypotheses 144:110280
Poljungreed I, Boonyarattanakalin S (2017) Dihydroxyacetone production by Gluconobacter frateurii in a minimum medium using fed-batch fermentation. J Chem Technol Biot 92(10):2635–2641
Prust C, Hoffmeister M, Liesegang H, Wiezer A, Fricke WF, Ehrenreich A, Gottschalk G, Deppenmeier U (2005) Complete genome sequence of the acetic acid bacterium Gluconobacter oxydans. Nat Biotechnol 23(2):195–200
Qin ZJ, Yang YT, Yu SQ, Liu L, Chen Y, Chen J, Zhou JW (2021) Repurposing the endogenous type I-E CRISPR/Cas system for gene repression in Gluconobacter oxydans WSH-003. ACS Synth Biol 10(1):84–93
Qin ZJ, Yu SQ, Chen J, Zhou JW (2022) Dehydrogenases of acetic acid bacteria. Biotechnol Adv 54:107863
Ripoll M, Jackson E, Trelles JA, Betancor L (2021) Dihydroxyacetone production via heterogeneous biotransformations of crude glycerol. J Biotechnol 340:102–109
Stasiak-Rozanska L, Blazejak S, Gientka I (2014) Effect of glycerol and dihydroxyacetone concentrations in the culture medium on the growth of acetic acid bacteria Gluconobacter oxydans ATCC 621. Eur Food Res Technol 239(3):453–461
Tateno H, Chen SY, Miseki Y, Nakajima T, Mochizuki T, Sayama K (2022) Photoelectrochemical oxidation of glycerol to dihydroxyacetone over an acid-resistant Ta:BiVO4 photoanode. ACS Sustain Chem Eng 10(23):7586–7594
Tian S, Liang X, Chen J, Zeng W, Zhou J, Du G (2020) Enhancement of 2-phenylethanol production by a wild-type Wickerhamomyces anomalus strain isolated from rice wine. Bioresource Technol 318:124257
Turner J, O’Loughlin DA, Green P, McDonald TO, Hamill KJ (2022) In search of the perfect tan: chemical activity, biological effects, business considerations, and consumer implications of dihydroxyacetone sunless tanning products. J Cosmet Dermatol-US. https://doi.org/10.1111/jocd.14968
Wang WL, Han FF, Li YG, Wu YS, Wang J, Pan RH, Shen GM (2014) Medium screening and optimization for photoautotrophic culture of Chlorella pyrenoidosa with high lipid productivity indoors and outdoors. Bioresource Technol 170:395–403
Wang PP, Xia Y, Li JH, Kang Z, Zhou JW, Chen J (2016) Overexpression of pyrroloquinoline quinone biosynthetic genes affects L-sorbose production in Gluconobacter oxydans WSH-003. Biochem Eng J 112:70–77
Wang P, Zeng W, Xu S, Du G, Zhou J, Chen J (2018) Current challenges facing one-step production of L-ascorbic acid. Biotechnol Adv 36(7):1882–1899
Westbrook AW, Miscevic D, Kilpatrick S, Bruder MR, Moo-Young M, Chou CP (2019) Strain engineering for microbial production of value-added chemicals and fuels from glycerol. Biotechnol Adv 37(4):538–568
Zeng W, Zhang H, Xu S, Fang F, Zhou J (2017) Biosynthesis of keto acids by fed-batch culture of Yarrowia lipolytica WSH-Z06. Bioresource Technol 243:1037–1043
Zeng W, Cai W, Liu L, Du G, Chen J, Zhou J (2019) Efficient biosynthesis of 2-keto-D-gluconic acid by fed-batch culture of metabolically engineered Gluconobacter japonicus. Synth Syst Biotechnol 4(3):134–141
Zhang Y, Sun Q, Liu Y, Cen XC, Liu DH, Chen Z (2021) Development of a plasmid stabilization system in Vibrio natriegens for the high production of 1,3-propanediol and 3-hydroxypropionate. Bioresour Bioprocess 8:125
We would like to express our gratitude to the National Natural Science Foundation of China for financial support.
This work was supported by the National Natural Science Foundation of China (Key Program, 31830068).
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Additional file 1
: Table S1. Primers used in this study. Table S2. Characteristic of 16 knocked out dehydrogenases.
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Zeng, W., Shan, X., Liu, L. et al. Efficient 1,3-dihydroxyacetone biosynthesis in Gluconobacter oxydans using metabolic engineering and a fed-batch strategy. Bioresour. Bioprocess. 9, 121 (2022). https://doi.org/10.1186/s40643-022-00610-7
- Gluconobacter oxydans
- Metabolic engineering
- Dehydrogenase genes
- Fed-batch fermentation