Skip to main content

Novel plasmid-free Gluconobacter oxydans strains for production of the natural sweetener 5-ketofructose



5-Ketofructose (5-KF) has recently been identified as a promising non-nutritive natural sweetener. Gluconobacter oxydans strains have been developed that allow efficient production of 5-KF from fructose by plasmid-based expression of the fructose dehydrogenase genes fdhSCL of Gluconobacter japonicus. As plasmid-free strains are preferred for industrial production of food additives, we aimed at the construction of efficient 5-KF production strains with the fdhSCL genes chromosomally integrated.


For plasmid-free 5-KF production, we selected four sites in the genome of G. oxydans IK003.1 and inserted the fdhSCL genes under control of the strong P264 promoter into each of these sites. All four recombinant strains expressed fdhSCL and oxidized fructose to 5-KF, but site-specific differences were observed suggesting that the genomic vicinity influenced gene expression. For further improvement, a second copy of the fdhSCL genes under control of P264 was inserted into the second-best insertion site to obtain strain IK003.1::fdhSCL2. The 5-KF production rate and the 5-KF yield obtained with this double-integration strain were considerably higher than for the single integration strains and approached the values of IK003.1 with plasmid-based fdhSCL expression.


We identified four sites in the genome of G. oxydans suitable for expression of heterologous genes and constructed a strain with two genomic copies of the fdhSCL genes enabling efficient plasmid-free 5-KF production. This strain will serve as basis for further metabolic engineering strategies aiming at the use of alternative carbon sources for 5-KF production and for bioprocess optimization.


The strictly aerobic acetic acid bacterium Gluconobacter oxydans contains at least eight membrane-bound dehydrogenases catalyzing the rapid chemo-, regio-, and stereoselective oxidation of sugars, alcohols, and polyols in the periplasm to organic acids, aldehydes, and ketones [1]. The resulting electrons are transferred via ubiquinone to the terminal cytochrome bo3 oxidase [2] or a cyanide-insensitive bd-type oxidase [3], both of which reduce oxygen to water. Due to the distinctive properties of the membrane-bound dehydrogenases, G. oxydans has become an important workhorse for oxidative biotransformations in biotechnology [4,5,6,7,8]. The first industrial application of G. oxydans was in vitamin C production via the Reichstein-Grüssner process [9], where the sorbitol dehydrogenase catalyzes the oxidation of D-sorbitol to L-sorbose [10]. Other products whose synthesis involves G. oxydans include dihydroxyacetone [11] or the anti-diabetic drug miglitol [12, 13].

Due to the vigorous incomplete periplasmic substrate oxidation of G. oxydans, only a small fraction of the carbon source is taken up into the cytoplasm and enters the central carbon metabolism, which is characterized by an incomplete glycolysis and an incomplete tricarboxylic acid (TCA) cycle [14]. Glucose is metabolized predominantly via the oxidative pentose phosphate pathway and to some extent via the Entner–Doudoroff pathway [15]. Pyruvate is partly converted to acetate as final product by pyruvate decarboxylase and acetaldehyde dehydrogenase [16]. As a consequence of the small fraction of substrate metabolized within the cell, the biomass yield of G. oxydans is quite low (about 0.1 g cell dry weight/g glucose). As this causes increased costs for biomass synthesis, metabolic engineering was used to create G. oxydans strains with improved biomass yield on glucose by reducing or avoiding its oxidation to gluconate [16, 17]. One of the resulting strains, IK003.1, which is derived from the parent strain 621H, lacks both the membrane-bound and the soluble glucose dehydrogenase as well as pyruvate decarboxylase. It has a 60% increased biomass yield on glucose and accumulates pyruvate instead of acetate [17].

Excess sugar consumption is associated with obesity and various diseases such as cardiovascular diseases or type II diabetes [18,19,20]. Thus, the food industry aims at the replacement of nutritive sugars such as sucrose or high-fructose corn syrup by non-nutritive sugar substitutes such as sucralose [21]. Various artificial and natural sweeteners are already available on the market, but most of them have drawbacks. Polyols such as d-sorbitol or d-xylitol show laxative effects [18], whereas compounds such as acesulfame K or steviol glycosides have a bitter off-taste [22]. 5-Keto-d-fructose (5-KF) is considered as a potential non-nutritive natural sweetener [23], which has been found e.g. in white wine [24, 25]. It shows a sweet taste quality identical to that of fructose and has a similar intrinsic sweet threshold concentration of 16.4 mmol/L [26]. Therefore, the development of processes for the production of 5-KF has recently gained attention.

G. oxydans is able to oxidize fructose to 5-KF when cultivated with fructose [25] or with mannitol, which is initially oxidized to fructose [27]. However, the enzyme responsible for 5-KF formation in G. oxydans is not known yet. In contrast, fructose dehydrogenase (FDH), a membrane-bound enzyme catalyzing the periplasmic oxidation of fructose to 5-KF with ubiquinone as electron acceptor, has been isolated and characterized from Gluconobacter japonicus NBRC3260 (formerly Gluconobacter industrius IFO3260) [28, 29]. It is a heterotrimeric enzyme composed of a small subunit with a putative Tat signal peptide (FdhS), a Sec-secreted cytochrome c subunit with three CXXCH motifs for covalent heme attachment and a C-terminal transmembrane helix anchoring the entire complex to the membrane (FdhC), and a large subunit with a covalently bound flavin adenine dinucleotide (FAD) cofactor (FdhL). It lacks a signal peptide and is presumably exported via the Tat system in complex with FdhS. The corresponding genes are organized in the polycistronic fdhSCL transcription unit [29]. Plasmid-based expression of the G. japonicus fdhSCL genes under the control of an adhAB promoter in a ΔadhA mutant of G. oxydans NBRC12528 lead to 20-fold higher FDH activity compared to G. japonicus wild-type cells, confirming the successful synthesis of FDH in this heterologous host [29].

The application of FDH for the targeted production of 5-KF was reported only recently [30]. A strain of G. oxydans 621H expressing the fdhSCL genes of G. japonicus under the control of the strong constitutive promoter P264 on the broad host range plasmid pBBR1p264-fdhSCL-ST showed good growth on fructose and formed 5-KF with a yield of 89 mol% 5-KF per fructose. Moreover, when combined with a second G. oxydans strain secreting the sucrase SacC of Zymomonas mobilis, this bacterial community was able to convert either purified sucrose or sucrose present in sugar beet extract to glucose and fructose and oxidize the latter to 5-KF with molar yields of > 90% and > 80%, respectively [30]. Most recently, 5-KF production from sucrose was reported for a G. oxydans strain with a chromosomal fdhSCL integration and plasmid-based expression of an invertase, resulting in conversion of 84 ± 2 mol% of the fructose units of sucrose into 5-KF [31]. G. oxydans carrying the expression plasmid pBBR1p264-fdhSCL-ST was also used for bioprocess development. When cultivated in a 2 L bioreactor with constant fructose feeding, 5-KF up to 489 g/L, yields up to 0.98 g 5-KF/g fructose and space-time yields up to 8.2 g/L/h were reached, demonstrating the efficiency of this 5-KF production process [26].

Considering an industrial implementation, 5-KF production with plasmid-free strains would be desirable. Therefore, the current study aimed at the development and characterization of G. oxydans strains with genomically integrated fdhSCL genes. Initially, four strains of G. oxydans IK003.1, each harboring a single copy of the fdhSCL genes at different genomic loci, were constructed and analyzed regarding 5-KF production. Based on these results, a strain carrying two genomic fdhSCL copies under control of the P264 promoter was constructed, which showed even better growth on fructose than the single-copy strains and formed 5-KF with yields of up to 0.82 g/g.

Results and discussion

Selection of genomic integration sites for the fdhSCL genes and design of integration constructs

In this study, we wanted to generate plasmid-free G. oxydans strains for the production of 5-KF by genomic integration of the FDH genes fdhSCL from G. japonicus. Because the genomic vicinity can influence the expression of integrated genes, we selected four different integration sites in the genome of G. oxydans IK003.1. For one of the insertions, the genes GOX2096-GOX2095 (GOX_RS11750) for a sorbitol dehydrogenase large subunit were replaced by the fdhSCL genes. GOX2096-GOX2095 represent an authentic frameshift in G. oxydans 621H leading to an inactive enzyme [14, 32]. Therefore, the replacement does not lead to a metabolic deficiency. In the case of the other three integration sites, the fdhSCL genes were inserted into intergenic regions (IGRs) without deleting any part of the genome. The IGRs were chosen based on the following criteria: (i) the genomic positions should be close to the origin of replication to profit from a positive gene dosage effect; (ii) the positions should be located between the 3′-ends of two convergent genes to avoid an interference with the regulation of neighboring genes; (iii) the expression levels of the adjacent genes should vary for the three sites to test the influence of the genomic vicinity on fdhSCL expression; (iv) the chromosomal gene upstream of the fdhSCL genes should possess a terminator to enable comparison of the three loci without readthrough from an upstream promoter. Applying those criteria and using RNAseq data [33] for the evaluation of the expression levels of the neighbouring genes, the following positions were selected: igr1 between GOX0013 and GOX0014, igr2 between GOX0028 and GOX0029, and igr3 between GOX0038 and GOX0039. The exact integration sites were positioned directly downstream of the terminator of the upstream gene, as predicted with the online tool ARNold [34].

The fdhSCL integration fragments were composed of 500 bp upstream DNA of the respective insertion site followed by the strong constitutive P264 promotor, the consensus ribosome binding site (RBS) AGGAG [33], the fdhSCL genes with an ATG start codon instead of TTG for fdhS, which was shown to be beneficial for 5-KF production [29], the bidirectional 100 bp terminator region downstream of GOX0028, which led to efficient termination according to RNA seq data [33], and 500 bp downstream DNA of the respective insertion site. The integration fragments were inserted into the suicide vector pAJ63a [35] and transferred into G. oxydans IK003.1 by conjugation, followed by a two-step homologous recombination protocol as outlined in the Methods section. The resulting integration strains were checked via colony-PCR and named IK003.1-igr1::fdhSCL, IK003.1-igr2::fdhSCL, IK003.1-igr3::fdhSCL, and IK003.1 Δsdh::fdhSCL (Fig. 1).

Fig. 1

Scheme of the loci used for targeted integration of the fdhSCL genes into the genome of G. oxydans IK003.1. Shown are the integration sites with the flanking genes, the P264 promoter (black arrow), a consensus RBS (black rectangle), the fdhSCL genes (gray arrows), and terminators (black hairpin = native, gray hairpin = inserted). The transcription strength of the flanking genes (strong, medium, weak) and the normalized read count (given by Fragments Per Kilobase of transcript per Million mapped reads (FPKM) values in brackets) are also indicated. FPKM values were determined via RNAseq with G. oxydans 621H grown on mannitol (exponential growth phase) [33]. To differentiate the transcription levels, the FPKM values (range of 0–446,627) were grouped in the lowest 25% (0–38, weak), the median 50% (38–318, medium) and the highest 25% (318–446,627, strong)

Shake flask cultivations with different G. oxydans IK003.1::fdhSCL strains with 18 g/L and 80 g/L fructose

Shake flask cultivations with offline sampling, using the four integration strains as well as IK003.1 as reference, were performed to assess whether the integration strains produce more 5-KF than the parental strain. Cultivations were performed with 18 g/L fructose (= 100 mM). Growth, fructose consumption, and 5-KF formation are shown in Fig. 2. After 29 h of cultivation, when no further growth was observed, IK003.1-igr3::fdhSCL, IK003.1-igr2::fdhSCL, and IK003.1 Δsdh::fdhSCL had completely consumed the fructose, resulting in higher 5-KF concentrations than observed for IK003.1-igr1::fdhSCL with 2.5 g/L residual fructose. The integration strains showed 15–22% higher growth rates (0.31 h−1 –0.33 h−1) than the reference strain IK003.1 (0.27 h−1) and reached higher final cell densities. Due to the lack of the fdhSCL genes, IK003.1 cannot generate energy by periplasmic fructose oxidation, which explains slower growth and lower biomass formation. Nevertheless, the reference strain produced small amounts of 5-KF, reaching a yield of 0.04 g/g. Low 5-KF production has also previously been described for G. oxydans grown on mannitol [27]. Here fructose oxidation to 5-KF was presumably catalyzed by the membrane-bound polyol dehydrogenase mSldAB, since a side activity for fructose oxidation has been described for a Gluconobacter thailandicus mSldAB homolog [36]. All integration strains formed 5-KF, but the kinetics differed (Fig. 2b). Strain IK003.1-igr3::fdhSCL showed the fastest 5-KF production, strains IK003.1-igr2::fdhSCL and IK003.1 Δsdh::fdhSCL were somewhat slower, and IK003.1-igr1::fdhSCL was much slower than the other strains. The 5-KF yields after 29 h were comparable for the three fastest strains (0.76 g/g for IK003.1-igr3::fdhSCL and IK003.1-igr2::fdhSCL, 0.74 g/g for IK003.1 Δsdh::fdhSCL), but lower for IK003.1-igr1::fdhSCL (0.61 g/g). This experiment already showed an influence of the integration site on 5-KF production with the ranking IK003.1-igr3::fdhSCL > IK003.1-igr2::fdhSCL > IK003.1 Δsdh::fdhSCL > IK003.1-igr1::fdhSCL. This ranking was later confirmed in additional experiments.

Fig. 2

Growth, 5-KF formation, and fructose consumption of the indicated G. oxydans strains in shake flasks. Depicted is a the cell density as OD600, b the 5-KF concentration, and c the fructose concentration determined by HPLC (method A). The strains were cultivated in 100 mL complex medium with 18 g/L fructose in 500 mL baffled shake flasks at 30 °C, 130 rpm, a shaking diameter of 50 mm, and 85% humidity. Shown are mean values of biological duplicates

To further investigate the four different integration sites, cultivations with online monitoring of respiratory activity in shake flasks were performed using the Respiration Activity MOnitoring System (RAMOS). Measuring the oxygen transfer rate (OTR) and the carbon dioxide transfer rate (CTR) provides extremely useful information about the metabolic activities and the physiological state of the microorganisms [37, 38]. 5-KF production from fructose is an oxidation reaction catalyzed by FDH and the electrons are transferred in the respiratory chain to oxygen as the final electron acceptor [26, 39]. Hence, 5-KF formation contributes to the OTR kinetics in addition to other catabolic activities of the G. oxydans strains. Cultivations with online monitoring of the respiratory activity were performed to obtain additional information on the growth behavior of the four integration strains using IK003.1 and the plasmid-containing strain IK003.1 pBBR1p264-fdhSCL-ST as reference (Additional file 1: Fig. S1). Increasing the fructose concentration from 18 g/L to 80 g/L led to a decrease of the 5-KF yield for all four integration strains, reaching values between 0.36 g/g and 0.58 g/g (Additional file 1: Table S1). Residual fructose concentrations of 25 g/L to 45 g/L were detected for the integration strains (Additional file 1: Table S1). IK003.1 pBBR1p264-fdhSCL-ST reached a much higher yield of 0.88 g/g.

The kinetics of OTR, CTR, and the respiratory quotient (RQ = CTR/OTR) observed for the six strains (Additional file 1: Fig. S1a–c) are likely caused by differences in the fructose oxidation rate, as a consequence of varying fdhSCL expression levels, which will be discussed below. The plasmid-containing strain IK003.1 pBBR1p264-fdhSCL-ST presumably has the highest FDH activity and showed the highest OTR. The maximal total oxygen consumption (TOC) of 220 mmol/L was reached already after 19 h (Additional file 1: Fig. S1d). Due to the rapid oxidation of fructose to 5-KF, less fructose is available for uptake and intracellular oxidation, resulting in the lowest total carbon dioxide evolution (TCE) of 50 mmol/L for IK003.1 pBBR1p264-fdhSCL-ST (Additional file 1: Fig. S1e). The reference strain IK003.1 had only a very low activity for fructose conversion to 5-KF and a very low maximal TOC of 80 mmol/L. The CTR was also quite low for IK003.1, because the strain may be energy-limited in the absence of FDH-based respiration, resulting in a maximal TCE of only 75 mmol/L. The 5-KF production of the four integration strains was slower than in the plasmid-based strain, resulting in a lower OTR. A maximal TOC of 250 mmol/L was reached for the integration strains at the end of the cultivation, except for IK003.1-igr1::fdhSCL. At the same time, more fructose was taken up and catabolized within the cell, resulting in higher CTR. The maximal TCE is two to four times higher for all integration strains in comparison with the plasmid-containing strain (Additional file 1: Fig. S1e). The kinetics of the RQ reflects these differences (Additional file 1: Fig. S1c).

Another parameter that probably influences the kinetics of OTR and CTR is the pH value. Strain IK003.1 forms pyruvate (pKa 2.49) instead of acetate (pKa 4.78), leading to a stronger acidification of the medium. In the experiment shown in Additional file 1: Fig. S1, pyruvate formation is dependent on the rate of intracellular fructose catabolism and thus should be reflected by the CTR value. Consequently, the integration strains should show a stronger acidification than the plasmid-containing strain and IK003.1, which was confirmed by the pH values measured after 29 h of cultivation (Additional file 1: Table S1). The pH influences the FDH activity and thus fructose consumption. The pH optimum for FDH is around 4 and activity decreases slightly at higher pH values, but strongly at lower pH, with no activity observed at pH 3 [29]. It is therefore likely that the OTR and CTR kinetics observed for the integration strains with a slow decrease after the maximum (Additional file 1: Fig. S1) and the incomplete fructose consumption (Additional file 1: Table S1) is caused by inhibition of FDH and other enzymes, such as those of the pentose phosphate pathway [40], due to acidification.

Influence of buffering on growth and 5-KF production during cultivation of IK003.1-igr1::fdhSCL with 80 g/L fructose in a RAMOS device

The decreasing pH during the cultivation had presumably a negative influence on growth and product formation during the cultivation. Therefore, it was investigated whether pH control has a positive effect on growth and product formation. CaCO3 is sometimes used in shake flask cultivations for buffering, but it has several disadvantages including turbidity of the medium [41]. Therefore, 2-(N-morpholino)ethansulfonic acid (MES) buffer with a pKa value of 6.1 was used [42]. Strain IK003.1-igr1::fdhSCL was chosen to compare cultivations without buffer and with 50 mM, 100 mM, and 150 mM MES buffer.

The addition of MES buffer had a strongly positive effect on 5-KF formation (Fig. 3). As expected, the pH value at the end of the cultivation increased from 3.3 for unbuffered cultivation to 4–4.7 for the cultivations with MES buffer (Fig. 3a). Fructose was completely consumed in the buffered cultures, resulting in a significantly increased 5-KF formation of up to 71 g/L and an increase of the yield from 0.56 g/g for the unbuffered culture to 0.86 g/g for the culture with 50 mM MES (Fig. 3a). At 100 mM and 150 mM MES, the 5-KF concentration and the yield were lower than at 50 mM MES, but the final OD600 was higher (4.1 for 0 mM MES, 4.9 for 50 mM MES, 5.4 for 100 mM MES, 5.9 for 150 mM MES). Higher pH values thus favor biomass formation and decrease 5-KF production.

Fig. 3

Cultivation of G. oxydans IK003.1-igr1::fdhSCL in a RAMOS device with 80 g/L fructose and different MES buffer concentrations. Depicted is a the residual fructose concentration (red), the 5-KF concentration (green), the yield g/g (grey), and the pH (blue), b the oxygen transfer rate (OTR) and c the total oxygen consumption (TOC). Cultivations were performed at 30 °C, 350 rpm, VL = 10 mL in 250 mL flasks, pHstart = 6 and a shaking diameter of 50 mm in complex medium with 80 g/L fructose and MES buffer at concentrations of 0 mM, 50 mM, 100 mM and 150 mM. Shown are mean values of duplicates and the concentrations determined for fructose and 5-KF in the two experiments as well as the resulting yields are shown as stars

The OTR kinetics of cultivations with the different MES concentrations showed clear differences (Fig. 3b). The maximal OTR of all MES-buffered cultures was about 50 mmol/L/h and thus 2.5-fold higher than for the unbuffered culture. At 100 mM and 150 mM MES, the OTR slowed down compared to 50 mM MES. This is most likely due to the higher osmolality of the medium, which increased from 0.56 Osmol/kg for unbuffered medium to 0.78 Osmol/kg for medium with 150 mM MES. The negative influence of osmolality on growth of G. oxydans has already been described [41, 43].

The kinetics of TOC is shown in Fig. 3c. As expected from the OTR kinetics, the TOC values of the MES-containing cultures were much higher than that of the unbuffered culture. Increasing MES concentrations correlated with increased TOC values, which can be explained by the fact that higher MES concentration led to higher biomass formation and thus a higher fraction of fructose was metabolized intracellularly, leading to more reducing equivalents per fructose than its simple oxidation to 5-KF.

Despite the increased lag phase, the positive effect of MES buffer regarding pH, TOC, OD600, and yield predominates. Therefore, subsequent shake flasks experiments were conducted with 150 mM MES buffer, which led to the highest TOC and the highest pH at the end of the cultivation. This was important for further experiments with fructose concentrations up to 210 g/L performed in shake flasks (Additional file 1: Fig. S5, Tab. S2).

Comparison of different G. oxydans strains during cultivation in a RAMOS device with 80 g/L fructose and 150 mM MES buffer

Based on the positive effect of MES buffering on 5-KF production by IK003.1-igr1::fdhSCL, these conditions were used to compare the four different integration strains among each other, with the parent strain IK003.1, and with the plasmid-containing strain IK003.1 pBBR1p264-fdhSCL-ST (Fig. 4).

Fig. 4

Cultivation of the indicated G. oxydans strains in a RAMOS device with 80 g/L fructose and 150 mM MES. Depicted is a the residual fructose concentration and the 5-KF concentration (determined by HPLC method B), the yield g/g, and the optical density (OD600) after 29 h, b the oxygen transfer rate (OTR), c the carbon dioxide transfer rate (CTR), and d the respiratory quotient (RQ, shown for OTR values above 5 mmol/L/h). The strains were cultivated in complex medium with 80 g/L fructose and 150 mM MES at 30 °C, 350 rpm, VL = 10 mL in 250 mL flasks, pHstart = 6 and a shaking diameter of 50 mm. Shown are mean values of duplicates and the values determined for optical density, the concentrations of fructose and 5-KF, and the resulting yields in the two experiments are shown as stars

As expected from the previous experiments, all strains except for IK003.1 consumed fructose completely and the final pH values varied between 4.3 and 4.6. 5-KF formation by the four integration strains was very similar (57–59 g/L), corresponding to yields of 0.71–0.75 g/g (Fig. 4a). Compared to the unbuffered cultures (Additional file 1: Table S1) this was an increase of 1.2- to 2-fold. The plasmid-containing strain formed 65 g/L 5-KF corresponding to a yield of 0.84 g/g.

The final OD600 of the integration strains ranged between 6.9 and 8.3 (Fig. 4a). In view of the comparable 5-KF formation of the four strains, these differences were unexpected and apparently are a consequence of the different genomic integration sites. The plasmid-containing strain had a much lower final OD600 of only 3.3 compared to the integration strains. As discussed above, this is caused by the higher copy number resulting in more fdhSCL transcript, resulting in faster fructose oxidation and a lower amount of fructose entering the cell. Additionally, a longer period of fructose oxidation by FDH also provides a longer period of energy supply for biomass formation from components of the yeast extract. Once fructose has been exhausted, growth is no longer sustained.

The statements made above are supported by the OTR and CTR kinetics (Fig. 4b, c). The plasmid-based strain reached its OTR maximum of 36 mmol/L/h already after 13 h, whereas the integration strains reached their maximum of ~ 55 mmol/L/h after 17 h –19 h (Fig. 4b). CTR was very low for the plasmid-based strain and much higher for the integration strains. This is in line with a higher intracellular fructose catabolism and a presumably higher consumption of yeast extract components (Fig. 4c). For strain IK003.1, both OTR and CTR were retarded compared to the integration strains. These kinetics are due to slow intracellular oxidation of fructose. In line with these data, the RQ value for IK003.1 was the highest of all strains (about 0.9), whereas the RQ of the plasmid-based strain was very low with a value of about 0.2. The integration strains showed RQ values in the range of 0.6–0.8 (Fig. 4d).

This experiment revealed that when using buffered conditions, the fdhSCL integration strains approached the 5-KF titer and the yield of the strain with plasmid-based fdhSCL expression. With respect to the four genomic integration sites, the differences in 5-KF titer and yield were rather small, but IK003.1-igr3::fdhSCL showed the fastest growth followed by IK003.1 Δsdh::fdhSCL and IK003.1-igr2::fdhSCL.

Scale up and fermentation in 2 L fermenter with IK003.1-igr3::fdhSCL

An important step for the industrial implementation of 5-KF production with a plasmid-free strain is the design and establishment of a suitable fermentation process. As a first step, a scale up from shake flasks to a 2 L fermenter was performed with strain IK003.1-igr3::fdhSCL, which was the best performing integration strain so far. To allow a direct comparison between shake flask (RAMOS system) and fermenter, the same medium, initial pH, and temperature were used for both cultivation devices. The shake flask was filled with inoculated medium by sterile transfer of a sample of the fermenter culture to ensure optimal comparability. In shake flask cultivations with 80 g/L fructose, no oxygen limitation was detected in the RAMOS devices. Hence, for a successful scale-up, oxygen limitation in the fermenter had to be avoided. For that reason, the dissolved oxygen tension (DOT) was kept above 30% by adjusting the agitation speed, whereas the aeration rate in the fermenter was kept constant at 1 vessel volume per minute (vvm). To verify the successful scale-up, online data (OTR, CTR, RQ) and offline data (OD600, pH, fructose and 5-KF concentration) were measured and compared. The results are shown in Additional file 1: Fig. S2. No significant differences in both, online and offline data, were found. Additional fermentations were performed as first optimization steps and confirmed the consistency of online and offline data (Additional file 1: Fig. S3 and Fig. S4). Hence, the scale up to a 2 L fermenter was successful and the process could be further optimized.

Higher product concentrations are desirable for an industrial application. To achieve higher 5-KF titers, the fructose concentration in batch fermentations was increased. To identify the optimal initial fructose concentration for the cultivation of IK003.1-igr3::fdhSCL, an experiment in shake flasks was performed using the RAMOS device and fructose concentrations between 80 g/L and 210 g/L. IK003.1-igr3::fdhSCL completely consumed fructose up to 210 g/L and the highest yield of 0.86 g/g was reached for the cultivation with 160 g/L fructose (Additional file 1: Fig. S5 and Table S2).

In a previous study, a 5-KF production process in a 2 L fermenter with the plasmid-based strain G. oxydans 621H pBBR1p264-fdhSCL-ST was described. This strain carried the same plasmid as IK003.1 pBBR1p264-fdhSCL-ST. G. oxydans 621H is not optimized for biomass formation from glucose and produces acetate rather than pyruvate. A batch fermentation with 150 g/L fructose was performed, reaching a 5-KF yield of 0.87 g/g [26]. To compare our genomic integration strain IK003.1-igr3::fdhSCL with this strain, a 2 L batch fermentation was performed under similar conditions (Fig. 5). An initial fructose concentration of 150 g/L was used to allow a direct comparison. Due to pH control by KOH addition, MES buffer was not included in the medium. The pH was set to 5, promoting both growth of G. oxydans and FDH activity. The DOT was maintained above 30% and antifoam was added twice during the cultivation. The OTR reached a maximum of 53 mmol/L/h after approx. 20 h and decreased sharply after 27 h, indicating the complete consumption of fructose (Fig. 5a). The OD600 increased over time and reached a final value of 9.2 (Fig. 5b), which is 1.7-fold higher compared with G. oxydans 621H pBBR1p264-fdhSCL-ST [26]. This difference is presumably caused by a somewhat higher fraction of fructose metabolized within the IK003.1 pBBR1p264-fdhSCL-ST cells and possibly also by the genetic alterations introduced into strain IK003.1 [17]. Most importantly, the 5-KF yield IK003.1-igr3::fdhSCL was 0.84 g/g and thus only slightly smaller than the 5-KF yield of 0.87 g/g determined for the plasmid-based strain [26].

Fig. 5

Cultivation of G. oxydans IK003.1-igr3::fdhSCL in a 2 L fermenter with pH control. Depicted is a the oxygen and carbon dioxide transfer rates (OTR and CTR), the respiratory quotient (RQ, shown for OTR values above 5 mmol/L/h), b optical density (OD600) and pH, c dissolved oxygen tension (DOT) and agitation speed, antifoam (AF) agent addition, and period of DOT control (indicated by arrows), d fructose and 5-KF concentrations. The cultivation was performed in complex medium with 150 g/L fructose with 1 L filling volume, DOT ≥ 30% controlled by agitation speed (500–1200 rpm), aeration rate (Q) =  L/min, T = 30 °C, pHcontrol ≥ 5

Shake flask cultivation of double integration strain IK003.1::fdhSCL2

The results described above were obtained with integration strains containing a single genomic fdhSCL copy and a resulting lower expression rate compared to plasmid-based fdhSCL expression (see below). To further improve the potential for plasmid-free 5-KF production, the double integration strain IK003.1::fdhSCL2 was constructed using the two most potent integration sites igr3 and igr2 for fdhSCL integration. The performance of this strain was compared to the parent single integration strains IK003.1-igr2::fdhSCL and IK003.1-igr3::fdhSCL and to the plasmid-based strain IK003.1 pBBR1p264-fdhSCL-ST in a shake flask experiment. Growth curves, fructose consumption, and 5-KF formation are shown in Fig. 6.

Fig. 6

Growth, 5-KF formation, and fructose consumption of the indicated G. oxydans strains. Depicted are a the growth as OD600, b the 5-KF and c the fructose concentration (determined by HPLC method A). The strains were cultivated in 100 mL complex medium with 18 g/L fructose in 500 mL baffled shake flasks at 30 °C, 130 rpm, a shaking diameter of 50 mm and 85% humidity. Shown are mean values of biological duplicates

The growth rate of strain IK003.1::fdhSCL2 (0.32 h−1) was close to that of the plasmid-based strain (0.33 h−1) and slightly higher than that of the single integration strains (0.28–0.29 h−1). The final OD600 after 30 h of the double integration strain (3.5) was lower than that of IK003.1-igr2::fdhSCL (4.1) and IK003.1-igr3::fdhSCL (4.1) and higher than that of the plasmid-based strain (2.3). Most importantly, the double integration strain IK003.1::fdhSCL2 was clearly faster than the single integration strains with respect to fructose consumption and 5-KF formation, but still slower than the plasmid-based strain. In a further experiment, the IK003.1::fdhSCL2 strain was compared with the parent single integration strains in a RAMOS cultivation device with 80 g/L fructose and 150 mM MES buffer (initial pH 6.0). As shown in Additional file 1: Fig. S6, the OTR kinetics confirmed faster fructose consumption by the double integration strain, reaching maximal OTR values at about 12 h, whereas the single integration strains reached the maximum after about 17 h. Under these conditions, IK003.1::fdhSCL2 reached a final 5-KF yield of 0.82 g/g, close to that of IK003.1 pBBR1p264-fdhSCL (0.84 g/g) obtained in the experiment shown in Fig. 4.

The properties of IK003.1::fdhSCL2 showed that doubling of the copy number of the fdhSCL genes and thus presumably a higher rate of fdhSCL transcription is sufficient to significantly increase the rate of fructose consumption and 5-KF formation. In the plasmid-based strain, the copy number of the fdhSCL genes is presumably above 20, as the copy number of the parent vector was determined to be 23 ± 6 in G. oxydanshsdR [44]. In this case, the increase in fdhSCL copy number did not lead to tenfold higher rates of fructose consumption and 5-KF production, showing that there were other factors that limit fructose oxidation.

Analysis of fdhSCL expression by RT-qPCR

To validate that different fdhSCL transcription levels are responsible for the phenotypic differences of single integration strains, reverse transcription quantitative PCR (RT-qPCR) was performed with the single integration strains, the double integration strain, and the plasmid-based strain using RNA from cells in the exponential growth phase. The gap gene (GOX0508), encoding glyceraldehyde 3–phosphate dehydrogenase, was tested as reference. It has been used as reference gene for RT-qPCR in G. oxydans before [45, 46]. However, with this reference gene we failed to detect the difference between single integration strains and the double integration strain, suggesting that gap expression is not constant under the experimental conditions employed and thus not a suitable reference gene (data not shown). We therefore used the gene for a ribosomal protein as reference, namely GOX0264 encoding the ribosomal protein L35. The results obtained for the fdhSCL/GOX0264 mRNA ratios are shown in Fig. 7, normalized to the mRNA ratio of the plasmid-based strain (5.03), which was set as 1.

Fig. 7

Relative fdhSCL transcript levels for the indicated G. oxydans strains as determined by RT-qPCR. Depicted is the transcript ratio fdhSCL/GOX0264 normalized to the transcript ratio of the plasmid-based strain IK003.1 pBBR1p264-fdhSCL-ST, which was set as 1.0. Shown are the mean values of at least three biological replicates and technical duplicates, with standard deviation as error bars

The fdh mRNA ratio of the four single integration strains varied between 3.5% and 6.6% of the value measured for the plasmid-based strain, which fits with a copy number of about 20 for pBBR1p264 in G. oxydans [44]. In the double integration strain, the fdh mRNA ratio was about twice as high (14% of the level of the plasmid-based strain), roughly corresponding to the sum of the values measured for IK003.1-igr2::fdhSCL and IK003.1-igr3::fdhSCL (12%). These results confirm the different expression levels expected from the fdhSCL copy numbers of the different strains. The fdhSCL transcription levels observed for the different integration strains correlated with the 5-KF production levels in the order IK003.1::fdhSCL2 > IK003.1-igr3::fdhSCL > IK003.1-igr2::fdhSCL > IK003.1 Δsdh::fdhSCL > IK003.1-igr1::fdhSCL.

Despite the usage of the same promoter and terminator structures, fdhSCL expression in the four different integration sites varied, indicating that the genomic vicinity of the target gene had an influence on the expression. It has been reported that RNA polymerase activity increases with proximity to the origin of replication [47] and that transcription speed is influenced by the codon composition [48]. However, both factors are not applicable to the differences observed here for the four single integration strains, since all four sites are close to the origin and contain the same DNA sequence. Genome architecture and DNA supercoiling are known to influence bacterial gene expression with DNA gyrase playing an important role by introducing negative supercoils or relaxing positive supercoils introduced by RNA polymerase [47, 49, 50]. In Escherichia coli, an increase in gyrase cleavage sites was found downstream of highly transcribed operons [51]. Furthermore, nucleoid-associated proteins influence DNA folding and gene expression [52, 53]. Such mechanisms, which have not been studied at all in G. oxydans, are likely to contribute to the variation in fdhSCL expression at the four different integration sites.


In this study, four different integration sites for heterologous genes were identified in the genome of G. oxydans, all enabling successful expression. The integration into the intergenic region of convergent genes flanked by terminators is thus a favorable option for future engineering studies requiring genomic expression of foreign genes. The position-dependent effects on gene expression observed in our experiments suggests that a comparison of different integration sites might be worthwhile. Chromosomal fdhSCL expression should enable stable expression and in fact we never observed loss of the ability for 5-KF production during growth for up to 30 generations and handling of the strains over several months. Furthermore, chromosomal expression avoids the necessity to use antibiotics required for plasmid-based fdhSCL expression. Plasmid loss can be an issue in the case of plasmid-based expression, however, no evidence for this has been observed in the case pBBR1p264-fdhSCL-ST. Another advantage of genomic fdhSCL expression is that it facilitates further metabolic engineering of the strains, for example toward utilization of alternative substrates. As doubling the genomic copy number of the fdhSCL genes correlated with twofold increased 5-KF synthesis rates, additional fdhSCL integrations could further increase 5-KF production. Also, the use of a promoter stronger than P264 could further enhance fdhSCL expression. Besides genetic optimization, process optimization is an obvious method to improve 5-KF production. In summary, our study provided the efficient G. oxydans strain IK003.1::fdhSCL2 for plasmid-free 5-KF production that will serve as basis for future strain and process development.


Strains, plasmids and oligonucleotides

All strains and plasmids used in this study are listed in Table 1. Oligonucleotides were obtained from Eurofins Genomics (Ebersberg, Germany) and are shown in Additional file 1: Table S3.

Table 1 Strains and plasmids used in this study

Media composition

G. oxydans strains were cultivated in complex medium containing 5 g/L yeast extract (Karl Roth GmbH, Karlsruhe, Germany or BD Biosciences, Heidelberg, Germany), 2.5 g/L MgSO4 × 7 H2O, 1 g/L (NH4)2SO4, 1 g/L KH2PO4. The initial pH was adjusted to 6 with KOH [54]. The media were supplemented with 50 µg/mL cefoxitin and 10 µM thymidine, and for plasmid-carrying strains 50 µg/mL kanamycin was added. For the precultures, 40 g/L mannitol was added as carbon source and main cultures were conducted with different fructose concentrations as indicated in the respective experiments. E. coli strains were cultivated in lysogeny broth-based media [55] at 37 °C and 130 rpm, and 50 µg/mL kanamycin was added for plasmid-carrying strains.

Generation of fdhSCL integration strains

To generate the fdhSCL integration strains, derivatives of pAJ63a [35] containing the fdhSCL genes of G. japonicus with promoter and terminator and flanked by about 500 bp DNA regions up- and downstream of the selected integration site were constructed. The required DNA fragments were amplified from suitable templates with the Phusion High Fidelity PCR Master Mix (New England Biolabs, Frankfurt am Main, Germany). The fdhSCL fragment with an ATG start codon for fdhS instead of the native TTG start codon was amplified from pBBR1p264-fdhSCL-ST [30] with the oligonucleotides RBS-ATG-fdhSCL-fwd, containing a consensus RBS, and fdhSCL-rev [33]. For all integration constructs, a 508 bp fragment covering the strong promoter of GOX0264 was amplified from pBBR1p264 [44] using the oligonucleotides P264-fwd and P264-rev-RBS-overlap with an overlap to the RBS and fdhS. A 100 bp bidirectional terminator region downstream of GOX0028 containing an overlap to fdhL was amplified with the oligonucleotides Term-GOX0028-fwd-fdhL-overlap and Term-GOX0028-rev from genomic DNA of strain IK003.1, which was isolated with the DNeasy Blood and Tissue Kit (Qiagen, Hilden, Germany). Two individual flanking regions of about 500 bp up- and downstream the respective integration sites were amplified from G. oxydans IK003.1 genomic DNA using specific oligonucleotide pairs with overlaps to the pAJ63a backbone, digested with PstI and KpnI, the promotor region and the terminator region to assemble all fragments via Gibson assembly [56]. The resulting fusion constructs were used to transform E. coli DH5α by the RbCl method [57]. Plasmids of positive clones were isolated using the QIAprep Spin Miniprep Kit (Qiagen, Hilden, Germany) and verified by sequencing (Eurofins Genomics, Ebersberg, Germany). Then the plasmids were transferred into the donor strain E. coli S17-1 for integration into G. oxydans IK003.1 via conjugation as described previously [17]. Positive clones, containing genomically integrated fdhSCL genes but not the vector backbone, were selected with 60 µg/mL 5-fluorouracile [35]. Positive clones were checked via colony PCR using a forward primer that binds upstream the upstream flanking region and a reverse primer, binding downstream of the downstream flanking region. Since the generation of the fdhSCL double integration strain turned out to be more challenging than the single integration strains, an adapted protocol was applied. IK003.1-igr2::fdhSCL was conjugated with E. coli S17–1 pAJ63a-igr3::fdhSCL according to the above mentioned protocol, while recombination media for the second recombination step and the agar plates for selecting the positive clones contained fructose instead of mannitol, as a strain with two chromosomal fdhSCL copies was assumed to show improved growth on fructose in comparison to a strain with a single fdhSCL copy. The double integration strain was obtained after several attempts.

Cultivation in regular shake flasks

For biological replicates, individual 10 mL-precultures in 100 mL unbaffled shake flasks with complex medium containing 40 g/L mannitol were inoculated from agar plates and incubated for about 24 h at 30 °C and 250 rpm. Cells from these precultures were harvested for 15 min at 20 °C and 5.000g, washed once in the main culture medium and used to inoculate 100 mL main cultures in 500 mL baffled shake flasks to an OD600 (optical density at 600 nm) of 0.15 in complex medium with 18 g/L (100 mM) fructose. Main cultures were incubated at 30 °C and 130 rpm with a shaking diameter of 50 mm and 85% humidity (Shaker ISF1-X, Kuhner, Birsfelden, Switzerland).

Cultivation in a respiration activity monitoring system (RAMOS)

Online monitoring of the respiratory activity in shake flask cultivations was performed using the Respiration Activity MOnitoring System (RAMOS) developed at the chair of biochemical engineering (RWTH Aachen University) [37, 38]. Commercial versions of the RAMOS device can be acquired from Kühner AG (Birsfeld, Switzerland) or HiTec Zang GmbH (Herzogenrath, Germany). Eight 250 mL shake flasks (unbaffled) were cultivated in parallel with an initial filling volume of 10 mL, 350 rpm shaking frequency and 50 mm shaking diameter (Climo-Shaker ISF1-X, Kuhner, Birsfelden, Switzerland). The aeration rate was set to 10 mL/min (1 vvm). Each flask is equipped with a partial pressure sensor for oxygen and a differential pressure sensor to determine oxygen and carbon dioxide transfer rates (OTR and CTR). The respiratory quotient (RQ) is the quotient of CTR and OTR. [37, 38]. For strain maintenance, glycerol stocks were used. Cells cultivated in complex medium with mannitol were harvested during the exponential growth phase, centrifuged and re-suspended in fresh preculture medium with 200 g/L glycerol. The glycerol stocks were stored at − 80 °C.

Precultures were inoculated with 100 µL glycerol stock suspension (OD600 = 2.4) and cultivated at 30 °C for 11 h to 19 h. Main cultures were inoculated from pre-cultures starting with an OD600 of 0.1. Preculture cells were centrifuged for 3 min at 16,214g and room temperature, and resuspended in main culture medium. Samples for offline analysis were taken from Erlenmeyer flasks operated at the same conditions in parallel to the online measurement. If necessary, 2-(N-morpholino) ethansulfonic acid (MES) buffer (pH 6, adjusted with 3 M KOH) was added in different concentrations to main cultures.

Cultivation in 2 L bioreactors

Fermentation experiments were performed in a 2 L Sartorius BIOSTAT® Bplus stirred tank reactor (Sartorius, Goettingen, Germany). The temperature was set to 30 °C and aeration was set to 1 L/min with a filling volume of 1 L (1 vvm). The fermenter was equipped with a six blade rusthton turbine and 4 baffles. During cultivation, the dissolved oxygen tension (DOT) was measured using a VisiFerm™ DO 225 pO2 sensor (Hamilton, Hoechst, Germany). The DOT was controlled at ≥ 30% by automatically adjusting the stirring rate between 500 rpm and 1500 rpm. The pH value was measured using a pH sensor (EasyFerm Plus K8 200, Hamilton, Hoechst, Germany). If necessary, pH was controlled with a 3 M KOH solution. Oxygen and carbon dioxide in the exhaust gas were measured using a DASGIP GA4 exhaust gas analyser (DASGIP, Eppendorf, Jülich, Germany). 0.5 mL antifoam agent Plurafac LF 1300 (BASF, Ludwigshafen, Germany) was added at the beginning of each experiment and when needed to prevent foaming. During fermentation, samples were taken from the bioreactor for offline analysis. Volume change by KOH titration and sampling were considered for mass balancing.

The performance of scale-up from shake flasks to the fermenter was investigated by cultivating simultaneously in both cultivation systems. For this purpose, media composition, pH, temperature and oxygen supply (aeration rate) were kept constant for both cultivation systems. The shake flasks were filled with medium from a fermenter. Cultivation broth was sterilely transferred from the fermenter into shake flasks to ensure that media composition, pH and optical density were identical [58,59,60].

Offline analyses

The optical density of cultures at 600 nm (OD600) was measured either with a Genesys 20 photometer (Thermo Scientific, Darmstadt, Germany) or with an Ultraspec 2100 UV–Visible Spectrophotometer (biochrom, Holliston MA, USA). The photometers have a linear range between 0.1 and 0.3 and samples were diluted with 0.9% (w/v) NaCl if necessary. The pH values were determined with a HI221 Basic pH (Hanna Instruments Deutschland GmbH, Vöhringen, Germany), which was calibrated using two standard buffer solutions at pH 4 and 7. The osmolality was determined using the cryoscopic Osmometer OSMOMAT® 030 (Genotec, Berlin, Germany).

Fructose consumption and 5-KF production were analyzed by HPLC of culture supernatants. 1 mL culture was centrifuged at 17,000g for 10 min and the supernatant was frozen at -20 °C until further analysis. Thawed samples were heated for 60 min at 60 °C (to avoid double peaks, probably caused by the existence of 5-ketofructose in an equilibrium of the keto and the germinal diol form [26]), filtered (0.2 µm syringe filter, Whatman™, GE Healthcare, Freiburg, Germany) and diluted with deionized water. Sugars were quantified using the same 5-KF standard with two different methods: HPLC method A: A 10 µL sample was measured in an Agilent LC-1100 system (Agilent, Santa Clara, CA, USA) equipped with a Carbo-Ca Guard Catridge (Phenomenex, Aschaffenburg, Germany) using a Rezex RCM-Monosaccharide 300, 7.8 mm column (Phenomenex, Aschaffenburg, Germany) for separation at 60 °C with water as eluent at a flow rate of 0.6 mL/min. 5-KF and fructose were detected with a refraction index detector (35 °C) [27]. 5-KF and fructose were calibrated in a range of 0.1 to 8 g/L, with retention times of 12.7 and 14.6 min, respectively. HPLC method B: An HPLC system of Shimadzu (Duisburg, Germany) was equipped with a precolumn Organic Acid Resin (40 × 8 mm, CS-Chromatographie Service, Langerwehe, Germany), the separating column Organic Acid Resin (250 × 8 mm, CS-Chromatographie Service, Langerwehe, Germany), and refraction index detector RID-20A (Shimadzu, Duisburg, Germany). The flow rate was set to 0.8 mL/min and an injection volume of 20 µL sample was used for analysis. 5 mM H2SO4 was used as mobile phase. Eluted components were detected and quantified using standard curves prepared with fructose and 5-KF solutions of known concentrations (0.032 g/L to 10 g/L). Evaporation during cultivations in the RAMOS device was determined gravimetrically and was taken into account for determination of fructose and 5-KF concentrations. Yields were calculated by dividing the produced 5-KF by the total fructose concentration and are indicated in g/g.

Analysis of gene expression by RT-qPCR

Strains were cultivated in shake flasks as described above and harvested in the exponential growth phase (after 7.25 h). 35 mL culture were mixed with 15 g ice, centrifuged for 5 min at 5.000g and 4 °C and the resulting cell pellet was shock-frozen in liquid nitrogen and stored at − 80 °C. RNA was isolated using QIAzol Lysis Reagent (Qiagen, Hilden, Germany) including the following steps: cell disruption in a Precellys 24 homogenizer (Bertin, Frankfurt am Main, Germany), chloroform extraction, isopropanol precipitation, an on-column DNA digest on RNeasy mini spin columns, with RNase-free DNase (Qiagen, Hilden, Germany). Purified RNA was subjected to a second DNA digest using the Ambion™ DNAfree™ DNA Removal Kit (Thermo Scientific, Waltham, MA USA). RNA was checked for integrity after the first or second DNase digest to exclude strong RNA degradation using a High Sensitivity RNA ScreenTape in the TapeStation 2200 (Agilent, Santa Clara, CA USA). Final RNA concentrations were determined using the Colibri microvolume spectrometer (Titerek-Berthold, Pforzheim, Germany).

cDNA was generated with SuperScript™ III Reverse Transcriptase (Thermo Scientific, Braunschweig, Germany) with the following protocol. 10 ng RNA, 150 ng random primers (Invitrogen, Thermo Scientific, Braunschweig, Germany) and 1 µL of 10 mM dNTP mix (Invitrogen, Thermo Scientific, Braunschweig, Germany) in a total volume of 14 µL were incubated for 5 min at 65 °C and cooled for 1 min at 4 °C. Subsequently, 4 µL 5× first strand buffer, 1 µL 0.1 mM DTT, and 1 µL SuperScript III reverse transcriptase were added and incubated for 5 min at 25 °C, 60 min at 50 °C and finally for 5 min at 70 °C for inactivation of reverse transcriptase. For all samples, additionally a no amplification control was generated with water instead of reverse transcriptase to exclude genomic DNA contaminations in RT-qPCR. RT-qPCR was performed with a qTower instrument (Analytik Jena, Jena, Germany) using KAPA SYBR FAST qPCR Master Mix (Roche Diagnostics, Mannheim, Germany). 2 µL of cDNA or no template control were used for RT-qPCR. For each sample, at least three biological replicates with two technical replicates were measured.

To set up RT-qPCR, primers were designed using the online tool Primer3plus [61] and default qPCR settings with a target PCR product of 100–120 bp and an annealing temperature of 60 °C. Three different primer pairs for fdhSCL, two binding in fdhS and one in fdhC, one primer pair for GOX0264, and three primer pairs for gap (GOX0508) were designed and tested for PCR specificity. To optimize RT-qPCR conditions, all primer pairs were compared in a gradient from 57.1 to 63.9 °C regarding PCR specificity via agarose gel electrophoresis and melting curve analysis. The optimal temperature was determined to be 57.1 °C. Subsequently, the PCR efficiency was determined by running a RT-qPCR with an 8-step 1:10 dilution series of cDNA. Ct values were determined using qPCRsoft 3.1 (Analytik Jena). The optimal primer pairs were selected to quantitatively amplify cDNA fragments of fdhC (q-fdhC-fwd + q-fdhC-rev, PCR efficiency of 103.2%), of GOX0264 (q-GOX0264-fwd + q-GOX0264-rev, 103%), and of GOX0508 (q-gap-fwd2 + q-gap-rev2, 91.8%) Relative transcript levels were calculated from Ct values, considering the primer efficiencies, and normalized to the transcript levels of the plasmid strain.

Availability of data and materials

The datasets supporting the conclusions of this article are included within the article and the additional file (Additional file1: Tables S1, S2, and S3, Figures S1, S2, S3, S4, S5, and S6).





Carbon dioxide transfer rate


Dissolved oxygen tension


Deoxyribonucleic acid


Flavin adenine dinucleotide


Fructose dehydrogenase


Fragments Per Kilobase of transcript per Million mapped reads


High-performance liquid chromatography


Intergenic regions


2-(N-Morpholino)ethansulfonic acid

OD600 :

Optical density at 600 nm


Origin of replication


Oxygen transfer rate


Respiration activity MOnitoring System


Ribosome binding site


Reverse transcription quantitative polymerase chain reaction


Respiratory quotient


Tricarboxylic acid cycle


Total carbon dioxide evolution


Total oxygen consumption


Vessel volume per minute


  1. 1.

    Matsushita K, Toyama H, Adachi O. Respiratory chains and bioenergetics of acetic acid bacteria. In: Rose AH, editor. Advances in Microbiol Physiology, vol. 36. Tempest DW: Academic Press; 1994. p. 247–301.

    Google Scholar 

  2. 2.

    Richhardt J, Luchterhand B, Bringer S, Büchs J, Bott M. Evidence for a key role of cytochrome bo3 oxidase in respiratory energy metabolism of Gluconobacter oxydans. J Bacteriol. 2013;195:4210–20.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  3. 3.

    Miura H, Mogi T, Ano Y, Migita CT, Matsutani M, Yakushi T, Kita K, Matsushita K. Cyanide-insensitive quinol oxidase (CIO) from Gluconobacter oxydans is a unique terminal oxidase subfamily of cytochrome bd. J Biochem. 2013;153:535–45.

    CAS  PubMed  Article  Google Scholar 

  4. 4.

    De Muynck C, Pereira CS, Naessens M, Parmentier S, Soetaert W, Vandamme EJ. The genus Gluconobacter oxydans: comprehensive overview of biochemistry and biotechnological applications. Crit Rev Biotechnol. 2007;27:147–71.

    PubMed  Article  CAS  Google Scholar 

  5. 5.

    Deppenmeier U, Hoffmeister M, Prust C. Biochemistry and biotechnological applications of Gluconobacter strains. Appl Microbiol Biotechnol. 2002;60:233–42.

    CAS  PubMed  Article  Google Scholar 

  6. 6.

    Gupta A, Singh VK, Qazi GN, Kumar A. Gluconobacter oxydans: its biotechnological applications. J Mol Microbiol Biotechnol. 2001;3:445–56.

    CAS  PubMed  Google Scholar 

  7. 7.

    Hölscher T, Schleyer U, Merfort M, Bringer-Meyer S, Görisch H, Sahm H. Glucose oxidation and PQQ-dependent dehydrogenases in Gluconobacter oxydans. J Mol Microbiol Biotechnol. 2009;16:6–13.

    PubMed  Article  CAS  Google Scholar 

  8. 8.

    Saichana N, Matsushita K, Adachi O, Frebort I, Frebortova J. Acetic acid bacteria: a group of bacteria with versatile biotechnological applications. Biotechnol Adv. 2015;33:1260–71.

    CAS  PubMed  Article  Google Scholar 

  9. 9.

    Reichstein T, Grüssner A. Eine ergiebige Synthese der l-Ascorbinsäure (C-vitamin). Helv Chim Acta. 1934;17:311–28.

    CAS  Article  Google Scholar 

  10. 10.

    Pappenberger G, Hohmann HP. Industrial production of l-ascorbic acid (vitamin C) and d-isoascorbic acid. Adv Biochem Eng Biotechnol. 2014;143:143–88.

    CAS  PubMed  Google Scholar 

  11. 11.

    Gätgens C, Degner U, Bringer-Meyer S, Herrmann U. Biotransformation of glycerol to dihydroxyacetone by recombinant Gluconobacter oxydans DSM 2343. Appl Microbiol Biotechnol. 2007;76:553–9.

    PubMed  Article  CAS  Google Scholar 

  12. 12.

    Ke X, Pan-Hong Y, Hu ZC, Chen L, Sun XQ, Zheng YG. Synergistic improvement of PQQ-dependent d-sorbitol dehydrogenase activity from Gluconobacter oxydans for the biosynthesis of miglitol precursor 6-(N-hydroxyethyl)-amino-6-deoxy-alpha-l-sorbofuranose. J Biotechnol. 2019;300:55–62.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  13. 13.

    Schedel M. Weiße biotechnologie bei Bayer healthcare product supply: mehr als 30 Jahre Erfahrung. Chem Ing Tec. 2006;78:485–9.

    CAS  Article  Google Scholar 

  14. 14.

    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.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  15. 15.

    Hanke T, Nöh K, Noack S, Polen T, Bringer S, Sahm H, Wiechert W, Bott M. Combined fluxomics and transcriptomics analysis of glucose catabolism via a partially cyclic pentose phosphate pathway in Gluconobacter oxydans 621H. Appl Environ Microbiol. 2013;79:2336–48.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  16. 16.

    Krajewski V, Simic P, Mouncey NJ, Bringer S, Sahm H, Bott M. Metabolic engineering of Gluconobacter oxydans for improved growth rate and growth yield on glucose by elimination of gluconate formation. Appl Environ Microbiol. 2010;76:4369–76.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  17. 17.

    Kiefler I, Bringer S, Bott M. Metabolic engineering of Gluconobacter oxydans 621H for increased biomass yield. Appl Microbiol Biotechnol. 2017;101:5453–67.

    CAS  PubMed  Article  Google Scholar 

  18. 18.

    Carocho M, Morales P, Ferreira I. Sweeteners as food additives in the XXI century: a review of what is known, and what is to come. Food Chem Toxicol. 2017;107:302–17.

    CAS  PubMed  Article  Google Scholar 

  19. 19.

    Hu FB, Malik VS. Sugar-sweetened beverages and risk of obesity and type 2 diabetes: epidemiologic evidence. Physiol Behav. 2010;100:47–54.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  20. 20.

    Yang Q, Zhang Z, Gregg EW, Flanders WD, Merritt R, Hu FB. Added sugar intake and cardiovascular diseases mortality among US adults. JAMA Intern Med. 2014;174:516–24.

    CAS  PubMed  Article  Google Scholar 

  21. 21.

    Mattes RD, Popkin BM. Nonnutritive sweetener consumption in humans: effects on appetite and food intake and their putative mechanisms. Am J Clin Nutr. 2009;89:1–14.

    CAS  PubMed  Article  Google Scholar 

  22. 22.

    Hellfritsch C, Brockhoff A, Stähler F, Meyerhof W, Hofmann T. Human psychometric and taste receptor responses to steviol glycosides. J Agric Food Chem. 2012;60:6782–93.

    CAS  PubMed  Article  Google Scholar 

  23. 23.

    Wyrobnik DH, Wyrobnik IH, Silcoff ER: Agent for reducing the useable calorie content of food and for therapeutic reduction of weight, in particular for use in the case of adiposity (obesity). Patent Application No. US 2009/0060956A1; 2009.

  24. 24.

    Blasi M, Barbe JC, Dubourdieu D, Deleuze H. New method for reducing the binding power of sweet white wines. J Agric Food Chem. 2008;56:8470–4.

    CAS  PubMed  Article  Google Scholar 

  25. 25.

    Barbe J-C, De Revel G, Joyeux A, Bertrand A, Lonvaud-Funel A. Role of botrytized grape micro-organisms in SO2 binding phenomena. J Appl Microbiol. 2001;90:34–42.

    CAS  PubMed  Article  Google Scholar 

  26. 26.

    Herweg E, Schöpping M, Rohr K, Siemen A, Frank O, Hofmann T, Deppenmeier U, Büchs J. Production of the potential sweetener 5-ketofructose from fructose in fed-batch cultivation with Gluconobacter oxydans. Bioresour Technol. 2018;259:164–72.

    CAS  PubMed  Article  Google Scholar 

  27. 27.

    Richhardt J, Bringer S, Bott M. Mutational analysis of the pentose phosphate and Entner–Doudoroff pathways in Gluconobacter oxydans reveals improved growth of a Δedd Δeda mutant on mannitol. Appl Environ Microbiol. 2012;78:6975–86.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  28. 28.

    Ameyama M, Shinagawa E, Matsushita K, Adachi O. d-Fructose dehydrogenase of Gluconobacter industrius - purification, characterization, and application to enzymatic micro-determination of d-Fructose. J Bacteriol. 1981;145:814–23.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  29. 29.

    Kawai S, Goda-Tsutsumi M, Yakushi T, Kano K, Matsushita K. Heterologous overexpression and characterization of a flavoprotein-cytochrome c complex fructose dehydrogenase of Gluconobacter japonicus NBRC3260. Appl Environ Microbiol. 2013;79:1654–60.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  30. 30.

    Siemen A, Kosciow K, Schweiger P, Deppenmeier U. Production of 5-ketofructose from fructose or sucrose using genetically modified Gluconobacter oxydans strains. Appl Microbiol Biotechnol. 2018;102:1699–710.

    CAS  PubMed  Article  Google Scholar 

  31. 31.

    Hoffmann JJ, Hovels M, Kosciow K, Deppenmeier U. Synthesis of the alternative sweetener 5-ketofructose from sucrose by fructose dehydrogenase and invertase producing Gluconobacter strains. J Biotechnol. 2020;307:164–74.

    CAS  PubMed  Article  Google Scholar 

  32. 32.

    Kranz A, Vogel A, Degner U, Kiefler I, Bott M, Usadel B, Polen T. High precision genome sequencing of engineered Gluconobacter oxydans 621H by combining long nanopore and short accurate Illumina reads. J Biotechnol. 2017;258:197–205.

    CAS  PubMed  Article  Google Scholar 

  33. 33.

    Kranz A, Busche T, Vogel A, Usadel B, Kalinowski J, Bott M, Polen T. RNAseq analysis of α-proteobacterium Gluconobacter oxydans 621H. BMC Genomics. 2018;19:24.

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  34. 34.

    Naville M, Ghuillot-Gaudeffroy A, Marchais A, Gautheret D. ARNold: a web tool for the prediction of Rho-independent transcription terminators. RNA Biol. 2011;8:11–3.

    CAS  PubMed  Article  Google Scholar 

  35. 35.

    Peters B, Junker A, Brauer K, Mühlthaler B, Kostner D, Mientus M, Liebl W, Ehrenreich A. Deletion of pyruvate decarboxylase by a new method for efficient markerless gene deletions in Gluconobacter oxydans. Appl Microbiol Biotechnol. 2013;97:2521–30.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  36. 36.

    Ano Y, Hours RA, Akakabe Y, Kataoka N, Yakushi T, Matsushita K, Adachi O. Membrane-bound glycerol dehydrogenase catalyzes oxidation of d-pentonates to 4-keto-d-pentonates, d-fructose to 5-keto-d-fructose, and d-psicose to 5-keto-d-psicose. Biosci Biotechnol Biochem. 2017;81:411–8.

    CAS  PubMed  Article  Google Scholar 

  37. 37.

    Anderlei T, Büchs J. Device for sterile online measurement of the oxygen transfer rate in shaking flasks. Biochem Eng J. 2001;7:157–62.

    CAS  PubMed  Article  Google Scholar 

  38. 38.

    Anderlei T, Zang W, Papaspyrou M, Büchs J. Online respiration activity measurement (OTR, CTR, RQ) in shake flasks. Biochem Eng J. 2004;17:187–94.

    CAS  Article  Google Scholar 

  39. 39.

    Deppenmeier U, Ehrenreich A. Physiology of acetic acid bacteria in light of the genome sequence of Gluconobacter oxydans. J Mol Microbiol Biotechnol. 2009;16:69–80.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  40. 40.

    Olijve W, Kok JJ. Analysis of growth of Gluconobacter oxydans in glucose containing media. Arch Microbiol. 1979;121:283–90.

    CAS  Article  Google Scholar 

  41. 41.

    Luchterhand B, Fischöder T, Grimm AR, Wewetzer S, Wunderlich M, Schlepütz T, Büchs J: Quantifying the sensitivity of G. oxydans ATCC 621H and DSM 3504 to osmotic stress triggered by soluble buffers. J Ind Microbiol Biotechnol 2015, 42:585-600.

    CAS  Article  Google Scholar 

  42. 42.

    Kandegedara A, Rorabacher DB. Noncomplexing tertiary amines as “better” buffers covering the range of pH 3–11. Temperature dependence of their acid dissociation constants. Anal Chem. 1999;71:3140–4.

    CAS  PubMed  Article  Google Scholar 

  43. 43.

    Kiefler I: Strain development of Gluconobacter oxydans: Complementation of non-functional metabolic pathways and increase of carbon flux. Dissertation, University of Düsseldorf, Germany. 2016.

  44. 44.

    Kallnik V, Meyer M, Deppenmeier U, Schweiger P. Construction of expression vectors for protein production in Gluconobacter oxydans. J Biotechnol. 2010;150:460–5.

    CAS  PubMed  Article  Google Scholar 

  45. 45.

    Schweiger P, Volland S, Deppenmeier U. Overproduction and characterization of two distinct aldehyde-oxidizing enzymes from Gluconobacter oxydans 621H. J Mol Microbiol Biotechnol. 2007;13:147–55.

    CAS  PubMed  Article  Google Scholar 

  46. 46.

    Meyer M, Schweiger P, Deppenmeier U. Effects of membrane-bound glucose dehydrogenase overproduction on the respiratory chain of Gluconobacter oxydans. Appl Microbiol Biotechnol. 2013;97:3457–66.

    CAS  PubMed  Article  Google Scholar 

  47. 47.

    Lal A, Dhar A, Trostel A, Kouzine F, Seshasayee AS, Adhya S. Genome scale patterns of supercoiling in a bacterial chromosome. Nat Commun. 2016;7:11055.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  48. 48.

    Großmann P, Lück A, Kaleta C. Model-based genome-wide determination of RNA chain elongation rates in Escherichia coli. Sci Rep. 2017;7:17213.

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  49. 49.

    Dorman CJ, Dorman MJ. DNA supercoiling is a fundamental regulatory principle in the control of bacterial gene expression. Biophys Rev. 2016;8:89–100.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  50. 50.

    El Houdaigui B, Forquet R, Hindré T, Schneider D, Nasser W, Reverchon S, Meyer S. Bacterial genome architecture shapes global transcriptional regulation by DNA supercoiling. Nucleic Acids Res. 2019;47:5648–57.

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  51. 51.

    Sutormin D, Rubanova N, Logacheva M, Ghilarov D, Severinov K. Single-nucleotide-resolution mapping of DNA gyrase cleavage sites across the Escherichia coli genome. Nucleic Acids Res. 2019;47:1373–88.

    CAS  PubMed  Article  Google Scholar 

  52. 52.

    Landick R, Wade JT, Grainger DC. H-NS and RNA polymerase: a love–hate relationship? Curr Opin Microbiol. 2015;24:53–9.

    CAS  PubMed  Article  Google Scholar 

  53. 53.

    Browning DF, Grainger DC, Busby SJW. Effects of nucleoid-associated proteins on bacterial chromosome structure and gene expression. Curr Opin Microbiol. 2010;13:773–80.

    CAS  PubMed  Article  Google Scholar 

  54. 54.

    Richhardt J, Bringer S, Bott M. Role of the pentose phosphate pathway and the Entner-Doudoroff pathway in glucose metabolism of Gluconobacter oxydans 621H. Appl Microbiol Biotechnol. 2013;97:4315–23.

    CAS  PubMed  Article  Google Scholar 

  55. 55.

    Bertani G. Studies on lysogenesis.I. The mode of phage liberation by lysogenic Escherichia coli. J Bacteriol. 1951;62:293–300.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  56. 56.

    Gibson DG. Enzymatic assembly of overlapping DNA fragments. Methods Enzymol. 2011;498:349–61.

    CAS  PubMed  Article  Google Scholar 

  57. 57.

    Hanahan D. Studies on transformation of Escherichia coli with plasmids. J Mol Biol. 1983;166:557–80.

    CAS  PubMed  Article  Google Scholar 

  58. 58.

    Seletzky JM, Noack U, Hahn S, Knoll A, Amoabediny G, Büchs J. An experimental comparison of respiration measuring techniques in fermenters and shake flasks: exhaust gas analyzer vs. RAMOS device vs. respirometer. J Ind Microbiol Biotechnol. 2007;34:123–30.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  59. 59.

    Seletzky JM, Noak U, Fricke J, Welk E, Eberhard W, Knocke C, Büchs J. Scale-up from shake flasks to fermenters in batch and continuous mode with Corynebacterium glutamicum on lactic acid based on oxygen transfer and pH. Biotechnol Bioeng. 2007;98:800–11.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  60. 60.

    Silberbach M, Maier B, Zimmermann M, Büchs J. Glucose oxidation by Gluconobacter oxydans: characterization in shaking-flasks, scale-up and optimization of the pH profile. Appl Microbiol Biotechnol. 2003;62:92–8.

    CAS  PubMed  Article  Google Scholar 

  61. 61.

    Untergasser A, Nijveen H, Rao X, Bisseling T, Geurts R, Leunissen JA. Primer3Plus, an enhanced web interface to Primer3. Nucleic Acids Res. 2007;35:W71–4.

    PubMed  PubMed Central  Article  Google Scholar 

  62. 62.

    Simon R, Priefer U, Pühler A. A broad host range mobilization system for in vivo genetic engineering: transposon mutagenesis in Gram negative bacteria. Bio/Technology. 1983;1:784–91.

    CAS  Article  Google Scholar 

Download references


This work was financially supported by the Bundesministerium für Bildung und Forschung (BMBF) within Project No. 031B0370 by grants given to Michael Bott (031B0370B) and Jochen Büchs (031B0370C).

Author information




SB designed and performed characterization and optimization experiments in shake flasks with online monitoring (RAMOS), scale up and fermentation experiments, analyzed the data and drafted the manuscript. KW constructed the integration strains, designed and performed the shake flask cultivations and the RT-qPCR, analyzed the data and drafted the manuscript. CI performed the scale up experiments. AK selected the integration sites. MP performed some of the shake flask cultivations with online monitoring. AW set up HPLC method A. MBo, JB and MBa supervised the study, assisted in data interpretation and participated in drafting the manuscript. All authors read and approved the final manuscript.

Corresponding authors

Correspondence to Jochen Büchs or Michael Bott.

Ethics declarations

Ethics approval and consent to participate

Not applicable.

Consent for publication

Not applicable.

Competing interests

The authors declare that they have no competing interest.

Additional information

Publisher's Note

Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Supplementary information

Additional file 1: Table S1. Offline data for cultivation of the indicated G. oxydans strains with 80 g/L fructose in a RAMOS device shown in Fig. S1. Table S2. Offline date for the cultivation of G. oxydans IK003.1-igr3::fdhSCL in a RAMOS device with different fructose concentrations shown in Fig. S5. Table S3. Oligonucleotides used in this study. Figure S1. Cultivation of the indicated G. oxydans strains with 80 g/L fructose in a RAMOS device with online monitoring. Depicted are (a) the oxygen transfer rate (OTR) (b) the carbon dioxide transfer rate (CTR) (c) the respiratory quotient (RQ shown for OTR values above 5 mmol/L/h), (d) the total oxygen consumption (TOC) and (e) the total carbon dioxide evolution (TCE). The strains were cultivated in complex medium with 80 g/L fructose at 30 °C, 350 rpm, VL = 10 mL in 250 mL flasks, pHstart = 6 and a shaking diameter of 50 mm. Shown are mean values of duplicates. Figure S2. Scale-up of batch fermentation of G. oxydans IK003.1-igr3::fdhSCL from shake flasks (RAMOS device) to a 2 L fermenter with 80 g/L fructose and 150 mM MES. Depicted are (a) oxygen transfer rate (OTR) and carbon dioxide transfer rate (CTR), (b) growth as OD600 and pH, (c) dissolved oxygen tension (DOT), agitation speed during fermentation, addition of antifoam agent (AF), and period of DOT control (indicated by arrows) and (d) fructose and 5-ketofructose concentration as determined by HPLC (method B). Cultivations were performed in complex medium with 80 g/L fructose prepared in the fermenter. The shake flask experiment was started with a sterile sample from the fermenter at 30 °C, 350 rpm, VL = 10 mL in 250 mL flasks, pHstart = 6 and a shaking diameter of 50 mm using the RAMOS system. Fermentation was performed with 1 L filling volume in a L fermenter, DOT was kept ≥ 30% by variation of the agitation speed (500–1250 rpm), aeration rate (Q) = 1 L/min, 30 °C. Figure S3. Cultivation of G. oxydans IK003.1-igr3::fdhSCL in a 2 L fermenter with 100 mM MES and 80 g/L fructose. Depicted is (a) the oxygen and carbon dioxide transfer rates (OTR and CTR), (b) optical density (OD600) and pH, (c) dissolved oxygen tension (DOT) and agitation speed, and (d) fructose and 5-ketofructose concentrations. The cultivation was performed with 1 L filling volume, DOT ≥ 30% controlled by agitation speed (500–1500 rpm), aeration rate (Q) = 1 L/min, T = 30 °C. Figure S4. Cultivation of G. oxydans IK003.1-igr3::fdhSCL in a 2 L fermenter with 80 g/L fructose and pH control. Depicted is (a) the oxygen and carbon dioxide transfer rates (OTR and CTR), (b) optical density (OD600) and pH, (c) dissolved oxygen tension (DOT) and agitation speed, and (d) fructose and 5-ketofructose concentrations. The cultivation was performed with 1 L filling volume, DOT ≥ 30% controlled by agitation speed (500–1500 rpm), aeration rate (Q) = 1 L/min, T = 30 °C. Figure S5. Cultivation of G. oxydans IK003.1-igr3::fdhSCL in a RAMOS device with different fructose concentrations and 150 mM MES (initial pH of 6). Depicted is the oxygen transfer rate during growth with the indicated concentrations of fructose in complex medium at 30 °C, 350 rpm, VL = 10 mL in 250 mL flasks, pHstart = 6 and a shaking diameter of 50 mm. Shown are mean values of duplicates. Figure S6. Cultivation of the indicated G. oxydans strains in a RAMOS device with 80 g/L fructose and 150 mM MES (initial pH of 6). Depicted is (a) the 5-ketofructose concentration (HPLC method B), the yield g/g, the OD600 and the final pH after 29 h and (b) the oxygen transfer rate (OTR). Cultivations were performed in complex medium with 80 g/L fructose and 150 mM MES buffer at 30 °C, 350 rpm, VL = 10 mL in 250 mL flasks, pHstart = 6 and a shaking diameter of 50 mm. Shown are mean values of duplicates.

Rights and permissions

Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons licence, and indicate if changes were made. The images or other third party material in this article are included in the article's Creative Commons licence, unless indicated otherwise in a credit line to the material. If material is not included in the article's Creative Commons licence and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this licence, visit The Creative Commons Public Domain Dedication waiver ( applies to the data made available in this article, unless otherwise stated in a credit line to the data.

Reprints and Permissions

About this article

Verify currency and authenticity via CrossMark

Cite this article

Battling, S., Wohlers, K., Igwe, C. et al. Novel plasmid-free Gluconobacter oxydans strains for production of the natural sweetener 5-ketofructose. Microb Cell Fact 19, 54 (2020).

Download citation


  • Gluconobacter oxydans
  • Sweetener
  • Chromosomal integration
  • 5-ketofructose
  • Fructose dehydrogenase