- Open Access
Understanding the interplay of carbon and nitrogen supply for ectoines production and metabolic overflow in high density cultures of Chromohalobacter salexigens
- María J. Salar-García†1, 3,
- Vicente Bernal†1, 4Email author,
- José M. Pastor1,
- Manuel Salvador2,
- Montserrat Argandoña2,
- Joaquín J. Nieto2,
- Carmen Vargas2 and
- Manuel Cánovas1Email author
© The Author(s) 2017
Received: 9 October 2016
Accepted: 1 February 2017
Published: 8 February 2017
The halophilic bacterium Chromohalobacter salexigens has been proposed as promising cell factory for the production of the compatible solutes ectoine and hydroxyectoine. This bacterium has evolved metabolic adaptations to efficiently grow under high salt concentrations by accumulating ectoines as compatible solutes. However, metabolic overflow, which is a major drawback for the efficient conversion of biological feedstocks, occurs as a result of metabolic unbalances during growth and ectoines production. Optimal production of ectoines is conditioned by the interplay of carbon and nitrogen metabolisms. In this work, we set out to determine how nitrogen supply affects the production of ectoines.
Chromohalobacter salexigens was challenged to grow in media with unbalanced carbon/nitrogen ratio. In C. salexigens, overflow metabolism and ectoines production are a function of medium composition. At low ammonium conditions, the growth rate decreased importantly, up to 80%. Shifts in overflow metabolism were observed when changing the C/N ratio in the culture medium. 13C-NMR analysis of ectoines labelling revealed a high metabolic rigidity, with almost constant flux ratios in all conditions assayed. Unbalanced C/N ratio led to pyruvate accumulation, especially upon N-limitation. Analysis of an ect − mutant demonstrated the link between metabolic overflow and ectoine biosynthesis. Under non ectoine synthesizing conditions, glucose uptake and metabolic overflow decreased importantly. Finally, in fed-batch cultures, biomass yield was affected by the feeding scheme chosen. High growth (up to 42.4 g L−1) and volumetric ectoine yields (up to 4.21 g L−1) were obtained by minimizing metabolite overflow and nutrient accumulation in high density cultures in a low nitrogen fed-batch culture. Moreover, the yield coefficient calculated for the transformation of glucose into biomass was 30% higher in fed-batch than in the batch culture, demonstrating that the metabolic efficiency of C. salexigens can be improved by careful design of culture feeding schemes.
Metabolic shifts observed at low ammonium concentrations were explained by a shift in the energy required for nitrogen assimilation. Carbon-limited fed-batch cultures with reduced ammonium supply were the best conditions for cultivation of C. salexigens, supporting high density growth and maintaining high ectoines production.
Compatible solutes are compounds that are accumulated in the cytoplasm of microorganisms to provide osmotic balance when exposed to osmotic stress [1, 2]. They are very soluble, low molecular weight, uncharged or zwitterionic organic compounds. Among compatible solutes, ectoine and its hydroxylated derivative hydroxyectoine are used as protectors of cells and tissues in pharmaceutical and cosmetic preparations (e.g. for skin protection) and stabilizers of enzymes and antibodies . Novel applications are underway, especially in biomedicine and biotechnology.
The chemical synthesis of ectoines is unaffordable at the industrial level due to the high cost of precursors (such as diaminobutyrate) and the chirality of the molecule, which makes microbial production the most feasible alternative . Ectoines biosynthesis shares the first steps with the aspartate family amino acid pathway [3, 5]. This pathway poses a challenge to cell homeostasis, since it is highly demanding in terms of carbon skeletons, metabolic energy and reducing equivalents, and evolution has driven the metabolism of natural producers towards optimality [6, 7].
Industrially acceptable microbial processes must have high yields and productivities. The development of efficient and economic biological processes with extremophiles is challenging due to both the technical difficulties associated with bioreactor operation  and the incomplete understanding of the physiology of the producing strains . This may lead to inefficient transformation of feedstocks, due to secondary products and low biomass yields due to growth inhibition [8, 9].
At the industrial level, ectoines are produced by the “bacterial milking” process, involving cycles of fed-batch fermentation of Halomonas elongata at 10–15% (w/v) NaCl to allow ectoine accumulation, followed by osmotic downshock at 2–3% (w/v) NaCl to release the osmolytes from the cells [4, 10, 11]. H. elongata has been engineered to increase ectoine productivity by deleting the ectoine uptake system and the degradation pathway . Chromohalobacter salexigens has been engineered to improve hydroxyectoine production at low temperature and salinity . Alternative processes for the production of osmolytes are based on fed-batch fermentation of Brevibacterium epidermis  or Halomonas boliviensis , continuous synthesis and excretion of osmolytes by recombinant mesophilic bacteria such as Escherichia coli [15–17] and Corynebacterium glutamicum  or halophilic bacteria such as Halomonas salina [19, 20]. On the other hand, Marinococcus M52 grown in a fed-batch microfiltration system provided elevated concentrations of hydroxyectoine .
Chromohalobacter salexigens (formerly, H. elongata) is a model halophilic γ-proteobacterium which accumulates ectoines as major compatible solutes . It has been proposed as an alternative ectoine(s) producer due to the extensive knowledge on its physiology and genetics, the availability of molecular tools for genetic manipulation and a sequenced genome . The synthesis of ectoines is regulated to cope with high environmental salt concentrations and other abiotic stress conditions such as high temperature [24–26]. We have recently described the adaptations undergone by its carbon metabolism to cope with high osmolarity. In this bacterium, glucose metabolism efficiency is a function of salt concentration. Ectoines biosynthesis at high salinity acts as a carbon sink and cell growth is slowed down due to the burden imposed. Moreover, overflow metabolism is minimized and biomass yield increases [6, 25]. At high salinity the cells balance their nitrogen content and ectoines are accumulated at the expense of proteins. Recent contributions to the field have taken advantage of metabolic modeling. A detailed reconstruction of the metabolism of ectoines in H. elongata was been recently published . The genome-scale reconstruction of the metabolism of C. salexigens  is not complete, since relevant pathways (such as ectoines catabolism) were not included and further discrepancies with experimental data have been identified (F. Piubeli, M. Argandoña, M. Salvador, J.J. Nieto and C. Vargas, personal communication).
Ectoines are a challenging target for metabolic engineers, since optimal production is conditioned by carbon and nitrogen metabolisms, and the interplay of nitrogen metabolism and ectoines production is unknown. In this work, we set out to determine its relevance for the production of ectoines. C. salexigens was challenged to grow in media with unbalanced carbon/nitrogen ratio. Shifts in growth, ectoines yield and metabolism were analyzed and used to design an efficient feeding scheme for fed-batch cultures. This study contributes to disclosing the principles below the efficiency of C. salexigens as an ectoines cell factory.
Bacterial strains and culture conditions
Chromohalobacter salexigens CHR61, a rifampicin resistant spontaneous mutant of C. salexigens DSM 3043T strain, and the ectoine synthesis deficient strain C. salexigens CHR62  (referred in the text as ect −) were used throughout this study.
Precultures were grown in SW-2 medium containing 2% (wt/vol) of total salts: 15.6 g L−1 NaCl, 4.07 g L−1 MgSO4·7H2O, 2.6 g L−1 MgCl2·6H2O, 0.4 g L−1 KCl, 67 mg L−1 CaCl2·2H2O, 47 mg L−1 NaBr and 13 mg L−1 NaHCO3 and 5 g L−1 of yeast extract . Cultures were started from frozen 20% glycerol stock cultures.
Glycerol stocks, solid culture media and precultures were supplemented with filter-sterilized rifampicine (Rf) to a final concentration of 25 μg mL−1.
For ectoines production and physiological studies, strains were cultured in M63 minimal medium (see below). Cultures were inoculated with late exponential phase SW-2 precultures, to an initial optical density (OD600nm) of 0.025 measured at 600 nm (Amersham Biosciences Novaspec Plus Visible Spectrophotometer, Uppsala, Sweden).
For physiological studies, cultures were grown in glucose M63 minimal medium (pH 7.2). Standard composition of medium was as follows: 20 mM, glucose, 16.3 g L−1 KH2PO4, 4.2 g L−1 KOH, 2 g L−1 (NH4)2SO4, 39.5 mg L−1 MgSO4·7H2O, 0.5 mg L−1 FeSO4·7H2O and 0.75–2.5 M NaCl . C. salexigens CHR61 was grown with 0.75–2.5 M NaCl, while the ectoine mutant strain CHR62 was studied at 0.75 M NaCl since it is not able to grow in higher salinities . Aerobic 100 mL batch cultures were grown in 0.5 L flasks incubated at 37 °C on a rotary shaker operated at 210 rpm.
The standard M63 medium was adapted by varying the concentrations of glucose and ammonium sulfate as described in the text, in order to analyze the effect of its composition on growth and ectoines production. Final glucose and ammonium concentration were varied to: (i) glucose concentration ranging from 10 to 100 mM with fixed 30 mM ammonium concentration and (ii) ammonium concentration ranging from 5 to 200 mM with a fixed 20 mM glucose concentration. Additionally, ammonium was substituted with 20 mM ectoine, alanine or glutamate to study the effect of organic nitrogen sources.
Bioreactor cultures: batch and fed-batch cultivation
High cell density cultures were performed in a Biostat B fermenter (Braun, Melsungen, Germany) with a 2 L vessel. Oxygen and pH were monitored with electrodes (Mettler-Toledo, Greifensee, Switzerland). Dissolved oxygen was maintained over 30% saturation by controlling air flow and stirring between 1 and 4 vvm and 40–1200 rpm, respectively. The pH was kept at 7.2 by automated addition of HCl/KOH.
For fed-batch cultivation, cells were initially cultured in the Biostat B system in batch for 16–20 h, to mid-exponential phase (initial volume: 1 L). Then, cells were fed following an exponential regime with glucose as the limiting nutrient. The feeding rate was controlled in order to limit the growth rate to a set value . For that aim, two concentrated medium feedings were designed with NaCl 2.5 M and 10- or 50-fold concentrated medium nutrients. The culture scheme was divided into two feeding phases consisting of 500 mL of the 10- and 50-fold medium, respectively, sequentially fed to the vessel. Final culture volume was 2 L.
To monitor culture growth, cells were resuspended in a NaCl solution (0.75–2.5 M). Absorbance was measured at 600 nm (Amersham Biosciences Novaspec Plus Visible Spectrophotometer, Uppsala, Sweden). OD600nm values and dry cell weight were correlated for the strain used. For that aim, samples were withdrawn at different times from cultures in M63 medium with 0.75 or 2.5 M NaCl. Cells were separated by filtration through 0.45 µm filters (Millipore Corp. Billerica, MA) and washed with a NaCl solution at the same concentration as in the growth medium. Filters were heat-dried to constant weight with Sartorius MA150 Moisture Analyzer (Sartorius AG, Göttingen, Germany). Cellular dry weight was correlated with OD600nm values: X (g L−1) = 0.5572·OD (NaCl, 0.75 M); X (g L−1) = 0.5322·OD (NaCl 2.5 M).
Analysis of extracellular metabolites by ion exchange HPLC-RI/UV
Extracellular metabolites (glucose, gluconate, pyruvate, acetate, lactate) were analyzed by HPLC (Shimadzu Scientific Instruments, Columbia, MD), equipped with differential refractive index and diode array detectors (Shimadzu Scientific Instruments, Columbia, MD), using a cation-exchange column (HPX-87H, BioRad Labs, Hercules, CA). The mobile phase was 5 mM H2SO4 at 0.5 mL min−1 flow rate and 45 °C.
Extraction and analysis of intracellular metabolites by reverse phase HPLC–UV
Compatible solutes were extracted from cell pellets by a variation of the method of Blight and Dyer . Briefly, cells were separated by centrifugation and stored at −20 °C until extracted. Cell pellets were dried in a Heto Vac VR-1 speedvac (Heto Lab Equipment, Allerod, Denmark), resuspended in 250 µL of methanol/chloroform/water mixture (10/5/4, v/v/v) and incubated for 15 min at 37 °C. To precipitate proteins and extract ectoines, 65 µL of chloroform and 65 µL of water were added. Liquid phases were separated by centrifugation and aqueous phase was separated, vacuum dried and reconstituted in H2O. Ectoine and hydroxyectoine were analyzed by HPLC as described elsewhere .
Spectrophotometric determination of glucose and ammonia
Glucose was determined by a glucose (HK) assay (Sigma Aldrich, Saint Louis, MO). Ammonium was analyzed by an assay based on glutamate dehydrogenase (R-Biopharm, Darmstadt, Germany). Measurements were performed in a 96-well microplate reader Synergy HT (Bio-Tek, Winooski, VT).
Isotopic labeling studies using 1H-NMR and 13C-NMR
For the labeling experiments, cells were batch grown in M63 medium with 20 mM [2-13C]glucose (CortecNet, Voisins-Le Bretonneux, France). Cells were harvested by centrifugation (16,000×g, 15 min, 4 °C) in the mid to late exponential phase (OD600nm 1.5–2). Compatible solutes (ectoines and glutamate) were extracted as previously explained. The aqueous extract was lyophilized and reconstituted in deuterated methanol. 1H-NMR and 13C-NMR spectra were recorded at 25 °C using Brucker AV400 and Brucker AV500 spectrometers at 400 and 500 MHz, respectively, and a relaxation time of 1 s in the case of 1H-NMR and 60 s for 13C-NMR. Peak areas were integrated for quantification. Flux ratios were estimated as previously described .
The M63 minimal medium used for physiological studies is optimized for C. salexigens balanced growth. In order to determine how this microorganism responds to perturbations in the carbon and nitrogen sources and identify dose–effect correlations, growth experiments were carried out by changing one individual medium component at a time while maintaining the other medium components constant. The effects of unbalanced carbon/nitrogen feeding on growth and ectoines production were assessed.
Effect of glucose on growth and production of ectoines
Effect of ammonium on growth and production of ectoines
Batch growth experiments were performed at 5–200 mM ammonium and a fixed concentration of glucose (20 mM). At low ammonium concentrations, both the biomass yield and the growth rate increased proportionally with ammonium supply. Low biomass yields are caused by the limited synthesis of cellular components and ectoines upon nitrogen limitation. Additionally, the effect on the growth rate suggests that ammonium assimilation may be affected by its actual concentration in the growth medium. A slight decrease of growth rate was observed at high ammonium concentrations (Fig. 1c). The rate of cell decay in the stationary phase increased dramatically at high ammonium concentration (data not shown), which suggests that it might exert toxic effects, especially upon carbon source exhaustion. Ectoine content of cells decreased at high ammonium concentrations, while volumetric titer reached a maximum at 30 mM ammonium (Fig. 1d).
Effects of ammonium availability on the metabolism of C. salexigens: carbon overflow and metabolic flux ratios
Unbalanced supply of glucose and ammonium might cause (i) metabolic shifts leading to overflow of by-products , or (ii) reduced availability of ammonium for ectoines and biomass synthesis. Inefficient growth correlated with the accumulation in the culture supernatant of gluconate, pyruvate and, to a lesser extent, acetate. The metabolite profiles were affected by the limiting nutrient. Gluconate and pyruvate accumulation was especially high in N-limited cultures, and continued after cell growth had been arrested. Metabolite overflow observed in C-limited cultures was much lower (Additional file 1: Table S1). At a constant initial glucose concentration, pyruvate production rate was greatly affected by ammonium availability, increasing proportionally to the C/N ratio in the medium.
Linking metabolic overflow and ectoine metabolism: the ect − mutant
Compatible solutes synthesis imposes a heavy metabolic burden which depends on salt concentration: at 2.5–3 M NaCl, ectoines make up to 16–24% of cell dry weight . Given the connection of glucose and ammonia supply to ectoines synthesis and metabolic overflow, we wondered what would be the metabolic overflow if ectoines were not produced. For that aim, the metabolic profile of the wild type C. salexigens CHR61 strain was compared to that of the ectoine-deficient CHR62 mutant (CHR62 lacks the ectABC genes; thus, it will be denoted as ect − mutant herein).
Metabolic overflow was also assessed in the ect − mutant. When growing on ammonium as nitrogen source, the ect − mutant showed an inefficient metabolism, with a high glucose consumption coefficient (YGlc/X) and a heavy accumulation of gluconate in the culture broth (Additional file 3: Table S2). Pyruvate and acetate overflow was similar for both strains, representing approximately 20% of the glucose consumed. Since the ect − mutant synthesized no ectoines, lower metabolic burden led to a 30% decrease in the glucose consumption rate. Despite this, gluconate accumulation rate was 9- to 12-fold higher, which suggests that in this mutant strain oxidation of glucose is not regulated to meet growth needs but, rather, responds to osmotic-stress  as demonstrated in mesophilic bacteria which do not produce compatible solutes [33, 34].
In the presence of 20 mM ectoine, both strains exhibited similar growth profiles. The specific rates of glucose consumption and pyruvate and gluconate production of wild type C. salexigens were lower than in the control medium (Additional file 3: Table S2). Thus, glucose consumption and production of gluconate and overflow metabolites are linked to the metabolic burden imposed by ectoine production. Acetate production increased, which might be result from ectoines degradation .
Linking metabolic overflow and nitrogen metabolism: the effect of the nitrogen source on growth
To further confirm the link between nitrogen assimilation pathways and metabolic burden, the wild type C. salexigens strain was grown in minimal medium with 2.5 M NaCl with four nitrogen sources: ammonia, ectoine, alanine and glutamate. The amino acids alanine and glutamate were selected since both are transformed to compounds of central metabolism closely related to ectoines biosynthesis and serve as nitrogen sources.
Similar growth profiles were observed in the presence of ectoine or glutamate as nitrogen sources, with shorter lag phase than in control cultures with ammonium as the sole nitrogen source. These results suggest that ammonia assimilation is a substantial contributor to the metabolic burden imposed by ectoine biosynthesis. A prolonged lag was observed in the growth on alanine (Fig. 3c), probably due to the accumulation of pyruvate and ammonia, formed during alanine degradation [35, 36].
Fed-batch cultivation of C. salexigens
In an attempt to find conditions to sustain high density cultivation and high ectoine titers, we decided to grow C. salexigens in glucose limited fed-batch cultures. The nutrient feeding profile was designed using glucose as the growth-limiting nutrient. After an initial batch phase, the culture was fed with a concentrated nutrient solution, fixing the growth rate through the feeding rate . Growth, production of ectoines and metabolites, and nutrient consumption were profiled along cultures.
Comparison of batch and fed-batch cultures of C. salexigens DSM 3043
Fed batch A
Fed batch B
Fed batch C
Set μ (h−1)
Initial [glucose] (mM)
Initial [ammonium] (mM)
Maximum biomass (g L−1)
2.12 ± 0. 2
12.6 ± 1. 6
28.1 ± 3.0
42.4 ± 2.0
Ectoine production (g L−1)
0.16 ± 0. 02
0.27 ± 0. 02
1.62 ± 0. 2
1.96 ± 0. 6
Hydroxyectoine production (g L−1)
0.18 ± 0. 02
0.18 ± 0. 03
1.51 ± 0. 3
2.25 ± 0. 7
Overall (gCDW g glucose −1 )
pO2 setting (%O2)
Aeration (L min−1)
Moreover, the yield coefficient calculated for the transformation of glucose into biomass was higher than in the batch culture. This demonstrates that overflow metabolism observed in batch cultures can be minimized in C-limited fed-batch, which is an indication that the metabolic efficiency of this microorganism can be improved by careful design of culture feeding schemes.
In this work we have shown the close relationship between nitrogen assimilation and ectoine production in C. salexigens. Engineering microbes for the production of nitrogenated compounds involve additional challenges, since both carbon and nitrogen metabolisms have to be rewired. Several cases of success have been reported, most of them for the biosynthesis of amino acids [37, 38].
While the growth rate of C. salexigens is not responsive to the concentration of glucose, it is greatly affected by ammonium. Both high and low ammonium concentrations affect growth and, interestingly, also ectoine production. In order to understand this behavior, central metabolism and the ectoine production pathway have to be jointly considered. For bacteria grown with ammonium as the nitrogen source, the building blocks for the biosynthesis of proteins, nucleic acids and all other nitrogen-containing cellular components derive from glutamate and glutamine . Two major systems have been described in bacteria for the incorporation of ammonium to the backbone of α-ketoglutarate (Fig. 3e). These pathways differ in substrate affinity and overall energy balance. The glutamine synthetase glutamate synthase (GS/GOGAT) system is the main pathway at low (<1 mM) ammonium concentrations, while glutamate dehydrogenase (GDH) is the main system at high concentrations. The GS/GOGAT system consumes one ATP equivalent per glutamate molecule synthesized .
The synthesis of ectoine and hydroxyectoine consumes glutamate as the donor of amino groups for the synthesis of aspartate (through aspartate aminotransferase) and l-2,4-diaminobutyrate (through EctB) (Fig. 3d) . In silico analysis of the metabolic network of H. elongata underlined that the use of either of these systems for ammonium uptake alters the overall stoichiometry of ectoine synthesis . In C. salexigens, which metabolizes glucose through the poor ATP-yielding Entner–Doudoroff pathway, this effect is even more pronounced, and ectoine synthesis leads to net consumption of ATP both at high and low ammonium concentration conditions. This is especially dramatic at low ammonium concentrations, since the GS/GOGAT pathway spends more cellular energy for nitrogen assimilation, lowering growth efficiency and forcing cells to balance the extra energy required to produce ectoines (Fig. 3f). At higher ammonium concentrations, ammonium is assimilated through the energetically less expensive GDH pathway.
Metabolism of C. salexigens adapts dynamically to varying energy requirements. Metabolic overflow was particularly sensitive to variations in ammonium availability; pyruvate and acetate are overflow metabolites, serving as readout of inefficient metabolism. Gluconate cannot be considered an overflow metabolite since it is produced by fast oxidation of glucose, an adaptation to gain advantage in the competition for carbon sources with microorganisms which are unable to use gluconate as carbon source . At a constant initial glucose concentration, pyruvate production rate increased proportionally to the C/N ratio in the medium, i.e. was higher as ammonium became more limiting. This suggests that at low ammonium conditions, glucose is incompletely oxidized to pyruvate to yield fast ATP to support the ATP-expensive ectoines biosynthesis pathway. Interestingly, this occurred without affecting central metabolism flux ratios reflecting the activity of the TCA cycle and the anaplerotic and ectoines biosynthesis pathways. A similar metabolic rigidity was previously observed in the response of C. salexigens to salt concentration  and it is further evidenced here in response to perturbations in the supply of nitrogen source. Apparently, environmental pressure has evolved a rigid metabolism to favor high ectoines biosynthetic fluxes at the expense of other adaptability strategies. Overflow metabolism may serve other roles. For instance, pyruvate overflow might feed other microbes in hypersaline environments .
In addition to their role as protecting agents, compatible solutes also are storage materials which can be used as carbon and nitrogen sources by microbes when environmental stresses decrease. This is also the case of ectoines, which can be used as carbon  and nitrogen sources (this work). Ectoines catabolism has been described in C. salexigens , Sinorhizobium meliloti and H. elongata  and Ruegeria pomeroyi . In C. salexigens and S. meliloti, it occurs through at least two systems with high similarities. Jebbar and col. identified an ectoine-induced operon involved in the uptake and catabolism of ectoine in S. meliloti (ehuABDC-eutABCD) . In C. salexigens, orthologues to some of these genes have been found, although their genomic organization is different . Ectoines catabolism yields acetate as end product. In fact, acetate was detected in the supernatants of ectoine supplemented cultures of wild type and ect − C. salexigens strains. Moreover, acetate overflow in C. salexigens is higher at low salt concentration , which might suggest that ectoines degradation might be regulated, while ectoines synthesis would be semi-constitutive. This hypothesis would explain the constant flux ratios assessed at different salinities .
The amino acids alanine and glutamate were selected for the nitrogen source experiments since both are readily metabolized yielding intermediaries of central metabolism, and nitrogenated precursors of ectoines synthesis . l-Glutamate is a nitrogen source for ectoines synthesis: transamination of l-glutamate yields l-aspartate (which is the precursor of ectoines synthesis) [3, 44–46] and l-glutamate is the nitrogen donor for the l-aspartate-β-semialdehyde to l-2,4-diaminobutyrate transformation (catalyzed by EctB) [3, 47]. In fact, glutamate is used as nitrogen source for the growth of many halophiles (see for instance ). In bacteria, l-alanine degradation occurs through oxidative deamination to pyruvate and ammonium . In C. salexigens, Csal2966 gene is annotated as alanine dehydrogenase . This reaction generates free ammonium to be used as nitrogen source , which assimilation is highly affected by its concentration in the medium (this work). This would explain why growth was delayed after M63 medium supplementation with alanine.
Although optimizing the production process was not the objective, the titers and productivities of ectoine reported herein are close to those previously reported with other halophiles [3, 14]. The best performance of C. salexigens was reported by Fallet et al.  using a continuous cultivation system consisting of a cascade of two continuously operated bioreactors. High cell density growth and ectoines production occurred in the first bioreactor, using cross-flow ultrafiltration for biomass retention. In the second bioreactor the cell broth was concentrated and subjected to an osmotic down-shock to force secretion of ectoines. With this system, they reported up to 61 g L−1 of biomass, 8.2 g L−1 of ectoines and a productivity of 2.1 g L−1 h−1.
Higher productivities of ectoines were assessed in cultures fed with low glucose and moderate ammonia levels. C. salexigens is adapted to thrive in nutrient poor environments, a phenomenon common to many other microorganisms, which usually exhibit high carbon overflow during growth on nutrient rich media. Low nutrient fluxes limit biomass produced, thus decreasing process productivity, especially with low nitrogen levels, which has an effect on the growth rate. Pyruvate and acetate overflow and gluconate accumulation might be avoided to ensure high productivities, and high biomass and specific ectoines yields should be reached to attain high levels of ectoines. In fed-batch cultures, growth rate was controlled using glucose as the limiting nutrient and ammonium content in the broth was adjusted in order to keep it within moderate values. The metabolism of C. salexigens was manipulated to avoid the activation of the ATP-expensive GS/GOGAT ammonium assimilation pathway and minimizing overflow metabolism. In fact, the overflow metabolism was only observed in the initial batch growth phase. Thus, further understanding the physiology of cell factories allows rationally developing high density fed-batch cultures and maximizing process productivities.
In this work, the importance of balanced carbon and nitrogen fluxes for optimal production of ectoines is demonstrated. The metabolism of C. salexigens is optimized to maximize the survival of the microorganism in nutrient limited systems and is highly inefficient in nutrient-rich environments, growth yield being limited by carbon overflow. The overflow metabolism shifts observed in C. salexigens with varying C/N ratios did not correlate with changes in flux ratios demonstrating the metabolic rigidity of C. salexigens. Finally, high density C. salexigens cultivation was possible with a low nitrogen feeding.
Designed the study: MJS, VB, MC. Performed the experiments: MJS, VB, JMP, MS. Performed NMR studies: JMP. Analyzed and discussed the data: MJS, VB, JMP, MS, MA, JJN, CV, MC. Drafted the manuscript: MJS, VB. All authors read and approved the final manuscript.
M.J. Gabaldón Martínez, M.D. Pardo Sánchez and Diego Martínez Pérez from Servicio Universitario de Instrumentación Científica (Universidad de Murcia) are acknowledged for their kind help with HPLC and NMR.
The authors declare that they have no competing interests.
Availability of data and materials
All data generated or analysed during this study are included in this published article and its supplementary information files.
This work has been partly funded by MICINN BIO2011-29233-C02-01, MINECO BIO2014-54411-C2-1-R (both including FEDER Funds), Junta de Andalucía project P11-CVI-7293 (EXTREMED) and by Fundación Séneca-CARM 08660/PI/08 and 19236/PI/14 projects. MICINN, MINECO, Junta de Andalucía and Fundación Séneca-CARM did not participate in the design of the study, collection, analysis, and interpretation of data or in writing the manuscript.
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- Oren A. Bioenergetic aspects of halophilism. Microbiol Mol Biol Rev. 1999;63:334–48.Google Scholar
- Brown AD. Microbial water stress physiology: principles and perspectives. 1st ed. New York: Wiley; 1990.Google Scholar
- Pastor JM, Salvador M, Argandoña M, Bernal V, Reina-Bueno M, Csonka LN, Iborra JL, Vargas C, Nieto JJ, Cánovas M. Ectoines in cell stress protection: uses and biotechnological production. Biotechnol Adv. 2010;28:782–801.View ArticleGoogle Scholar
- Kunte HJ, Lentzen G, Galinski EA. Industrial production of the cell protectant ectoine: protection mechanisms, processes, and products. Curr Biotechnol. 2014;3:10–25.View ArticleGoogle Scholar
- Vargas C, Argandoña M, Reina-Bueno M, Rodríguez-Moya J, Fernández-Aunión C, Nieto JJ. Unravelling the adaptation responses to osmotic and temperature stress in Chromohalobacter salexigens, a bacterium with broad salinity tolerance. Saline Syst. 2008;4:14.View ArticleGoogle Scholar
- Pastor JM, Bernal V, Salvador M, Argandoña M, Vargas C, Csonka L, Sevilla A, Iborra JL, Nieto JJ, Cánovas M. Role of central metabolism in the osmoadaptation of the halophilic bacterium Chromohalobacter salexigens. J Biol Chem. 2013;288:17769–81.View ArticleGoogle Scholar
- Schwibbert K, Marin-Sanguino A, Bagyan I, Heidrich G, Lentzen G, Seitz H, Rampp M, Schuster SC, Klenk H-P, Pfeiffer F, Oesterhelt D, Kunte HJ. A blueprint of ectoine metabolism from the genome of the industrial producer Halomonas elongata DSM 2581T. Environ Microbiol. 2011;13:1973–94.View ArticleGoogle Scholar
- Deive FJ, López E, Rodríguez A, Longo MA, Sanromán MÁ. Targeting the production of biomolecules by extremophiles at bioreactor scale. Chem Eng Technol. 2012;35:1565–75.View ArticleGoogle Scholar
- Schiraldi C, De Rosa M. The production of biocatalysts and biomolecules from extremophiles. Trends Biotechnol. 2002;20:515–21.View ArticleGoogle Scholar
- Sauer T, Galinski EA. Bacterial milking: a novel bioprocess for production of compatible solutes. Biotechnol Bioeng. 1998;57:306–13.View ArticleGoogle Scholar
- Tanimura K, Nakayama H, Tanaka T, Kondo A. Ectoine production from lignocellulosic biomass-derived sugars by engineered Halomonas elongata. Bioresour Technol. 2013;142:523–9.View ArticleGoogle Scholar
- Rodríguez-Moya J, Argandoña M, Iglesias-Guerra F, Nieto JJ, Vargas C. Temperature- and salinity-decoupled overproduction of hydroxyectoine by Chromohalobacter salexigens. Appl Environ Microbiol. 2013;79:1018–23.View ArticleGoogle Scholar
- Onraedt AE, Walcarius BA, Soetaert WK, Vandamme EJ. Optimization of ectoine synthesis through fed-batch fermentation of Brevibacterium epidermis. Biotechnol Prog. 2005;21:1206–12.View ArticleGoogle Scholar
- Van-Thuoc D, Guzmán H, Quillaguamán J, Hatti-Kaul R. High productivity of ectoines by Halomonas boliviensis using a combined two-step fed-batch culture and milking process. J Biotechnol. 2010;147:46–51.View ArticleGoogle Scholar
- Schubert T, Maskow T, Benndorf D, Harms H, Breuer U. Continuous synthesis and excretion of the compatible solute ectoine by a transgenic, nonhalophilic bacterium. Appl Environ Microbiol. 2007;73:3343–7.View ArticleGoogle Scholar
- Bestvater T, Louis P, Galinski EA. Heterologous ectoine production in Escherichia coli: by-passing the metabolic bottle-neck. Saline Syst. 2008;4:12.View ArticleGoogle Scholar
- He Y-Z, Gong J, Yu H-Y, Tao Y, Zhang S, Dong Z-Y. High production of ectoine from aspartate and glycerol by use of whole-cell biocatalysis in recombinant Escherichia coli. Microb Cell Fact. 2015;14:55.View ArticleGoogle Scholar
- Becker J, Schäfer R, Kohlstedt M, Harder BJ, Borchert NS, Stöveken N, Bremer E, Wittmann C. Systems metabolic engineering of Corynebacterium glutamicum for production of the chemical chaperone ectoine. Microb Cell Fact. 2013;12:110.View ArticleGoogle Scholar
- Zhang L, Lang Y, Nagata S. Efficient production of ectoine using ectoine-excreting strain. Extremophiles. 2009;13:717–24.View ArticleGoogle Scholar
- Lang Y, Bai L, Ren Y, Zhang L, Nagata S. Production of ectoine through a combined process that uses both growing and resting cells of Halomonas salina DSM 5928T. Extremophiles. 2011;15:303–10.View ArticleGoogle Scholar
- Schiraldi C, Maresca C, Catapano A, Galinski EA, De Rosa M. High-yield cultivation of Marinococcus M52 for production and recovery of hydroxyectoine. Res Microbiol. 2006;157:693–9.View ArticleGoogle Scholar
- Arahal DR, García MT, Vargas C, Cánovas D, Nieto JJ, Ventosa A. Chromohalobacter salexigens sp. nov., a moderately halophilic species that includes Halomonas elongata DSM 3043 and ATCC 33174. Int J Syst Evol Microbiol. 2001;51(Pt 4):1457–62.View ArticleGoogle Scholar
- Copeland A, O’Connor K, Lucas S, Lapidus A, Berry KW, Detter JC, Del Rio TG, Hammon N, Dalin E, Tice H, Pitluck S, Bruce D, Goodwin L, Han C, Tapia R, Saunders E, Schmutz J, Brettin T, Larimer F, Land M, Hauser L, Vargas C, Nieto JJ, Kyrpides NC, Ivanova N, Göker M, Klenk H-P, Csonka LN, Woyke T. Complete genome sequence of the halophilic and highly halotolerant Chromohalobacter salexigens type strain (1H11(T)). Stand Genomic Sci. 2011;5:379–88.View ArticleGoogle Scholar
- Canovas D, Vargas C, Csonka L, Ventosa A, Nieto J. Osmoprotectants in Halomonas elongata: high-affinity betaine transport system and choline–betaine pathway. J Bacteriol. 1996;178:7221–6.View ArticleGoogle Scholar
- Salvador M, Argandoña M, Pastor JM, Bernal V, Cánovas M, Csonka LN, Nieto JJ, Vargas C. Contribution of RpoS to metabolic efficiency and ectoines synthesis during the osmo- and heat-stress response in the halophilic bacterium Chromohalobacter salexigens. Environ Microbiol Rep. 2015;7:301–11.View ArticleGoogle Scholar
- Poolman B, Glaasker E. Regulation of compatible solute accumulation in bacteria. Mol Microbiol. 1998;29:397–407.View ArticleGoogle Scholar
- Ates O, Oner ET, Arga KY. Genome-scale reconstruction of metabolic network for a halophilic extremophile, Chromohalobacter salexigens DSM 3043. BMC Syst Biol. 2011;5:12.View ArticleGoogle Scholar
- Canovas D, Vargas C, Iglesias-Guerra F, Csonka LN, Rhodes D, Ventosa A, Nieto JJ. Isolation and characterization of salt-sensitive mutants of the moderate halophile Halomonas elongata and cloning of the ectoine synthesis genes. J Biol Chem. 1997;272:25794–801.View ArticleGoogle Scholar
- Vargas C, Coronado MJ, Ventosa A, Nieto JJ. Host range, stability and compatibility of broad host-range-plasmids and a shuttle vector in moderately halophilic bacteria. evidence of intrageneric and intergeneric conjugation in moderate halophiles. Syst Appl Microbiol. 1997;20:173–81.View ArticleGoogle Scholar
- Csonka LN. A third l-proline permease in Salmonella typhimurium which functions in media of elevated osmotic strength. J Bacteriol. 1982;151:1433–43.Google Scholar
- Nielsen J. Microbial process kinetics. In: Ratledge C, Christiansen B, editors. Basic biotechnol. 3rd ed. Cambridge: Cambridge University Press; 2006. p. 155–80.View ArticleGoogle Scholar
- Bligh EG, Dyer WJ. A rapid method of total lipid extraction and purification. Can J Biochem Physiol. 1959;37:911–7.View ArticleGoogle Scholar
- Metris A, George SM, Mulholland F, Carter AT, Baranyi J. Metabolic shift of Escherichia coli under salt stress in the presence of glycine betaine. Appl Environ Microbiol. 2014;80:4745–56.View ArticleGoogle Scholar
- Cánovas M, Bernal V, Sevilla A, Torroglosa T, Iborra JL. Salt stress effects on the central and carnitine metabolisms of Escherichia coli. Biotechnol Bioeng. 2007;96:722–37.View ArticleGoogle Scholar
- McFall E, Newman EB. Amino acids as carbon sources. In: Escherichia coli Salmonella Cell Mol Biol. 1996. p. 358–79.Google Scholar
- Reitzer LJ. Ammonia assimilation and the biosynthesis of glutamine, glutamate, aspartate, asparagine, l-alanine and d-alanine. In: Curtiss III R, Ingraham JL, Lin EC, Low Jr KB, Magasanik B, Reznikoff WS, Riley M, Schaechter M, Umbarger HE, editors. Escherichia coli Salmonella, Mol Cell Biol. 2nd ed. Washington, DC: ASM Press; 1996. p. 391–497.Google Scholar
- Wendisch VF. Microbial production of amino acids and derived chemicals: synthetic biology approaches to strain development. Curr Opin Biotechnol. 2014;30:51–8.View ArticleGoogle Scholar
- Hirasawa T, Shimizu H. Recent advances in amino acid production by microbial cells. Curr Opin Biotechnol. 2016;42:133–46.View ArticleGoogle Scholar
- Chavarría M, Kleijn RJ, Sauer U, Pflüger-Grau K, de Lorenzo V. Regulatory tasks of the phosphoenolpyruvate–phosphotransferase system of Pseudomonas putida in central carbon metabolism. MBio. 2012;3:e00028–12.View ArticleGoogle Scholar
- Oren A. Pyruvate: a key nutrient in hypersaline environments? Microorganisms. 2015;3:407–16.View ArticleGoogle Scholar
- Vargas C, Jebbar M, Carrasco R, Blanco C, Calderón MI, Iglesias-Guerra F, Nieto JJ. Ectoines as compatible solutes and carbon and energy sources for the halophilic bacterium Chromohalobacter salexigens. J Appl Microbiol. 2006;100:98–107.View ArticleGoogle Scholar
- Schulz A, Stöveken N, Binzen IM, Hoffmann T, Heider J, Bremer E. Feeding on compatible solutes: a substrate-induced pathway for uptake and catabolism of ectoines and its genetic control by EnuR. Environ Microbiol. 2016. doi:10.1111/1462-2920.13414.Google Scholar
- Jebbar M, Sohn-Bösser L, Bremer E, Bernard T, Blanco C. Ectoine-induced proteins in Sinorhizobium meliloti include an ectoine ABC-type transporter involved in osmoprotection and ectoine catabolism. J Bacteriol. 2005;187:1293–304.View ArticleGoogle Scholar
- Caspi R, Billington R, Ferrer L, Foerster H, Fulcher CA, Keseler IM, Kothari A, Krummenacker M, Latendresse M, Mueller LA, Ong Q, Paley S, Subhraveti P, Weaver DS, Karp PD. The MetaCyc database of metabolic pathways and enzymes and the BioCyc collection of pathway/genome databases. Nucleic Acids Res. 2016;44:D471–80.View ArticleGoogle Scholar
- Peters P. The biosynthesis of ectoine. FEMS Microbiol Lett. 1990;71:157–62.View ArticleGoogle Scholar
- Lo C-C, Bonner CA, Xie G, D’Souza M, Jensen RA. Cohesion group approach for evolutionary analysis of aspartokinase, an enzyme that feeds a branched network of many biochemical pathways. Microbiol Mol Biol Rev. 2009;73:594–651.View ArticleGoogle Scholar
- Cánovas D, Vargas C, Calderón MI, Ventosa A, Nieto JJ. Characterization of the genes for the biosynthesis of the compatible solute ectoine in the moderately halophilic bacterium Halomonas elongata DSM 3043. Syst Appl Microbiol. 1998;21:487–97.View ArticleGoogle Scholar
- Fallet C, Rohe P, Franco-Lara E. Process optimization of the integrated synthesis and secretion of ectoine and hydroxyectoine under hyper/hypo-osmotic stress. Biotechnol Bioeng. 2010;107:124–33.View ArticleGoogle Scholar