- Open Access
Production of the short peptide surfactant DAMP4 from glucose or sucrose in high cell density cultures of Escherichia coli BL21(DE3)
© Bruschi et al.; licensee BioMed Central Ltd. 2014
- Received: 9 April 2014
- Accepted: 26 June 2014
- Published: 19 August 2014
Peptides are increasingly used in industry as highly functional materials. Bacterial production of recombinant peptides has the potential to provide large amounts of renewable and low cost peptides, however, achieving high product titers from Chemically Defined Media (CDM) supplemented with simple sugars remains challenging.
In this work, the short peptide surfactant, DAMP4, was used as a model peptide to investigate production in Escherichia coli BL21(DE3), a classical strain used for protein production. Under the same fermentation conditions, switching production of DAMP4 from rich complex media to CDM resulted in a reduction in yield that could be attributed to the reduction in final cell density more so than a significant reduction in specific productivity. To maximize product titer, cell density at induction was maximized using a fed-batch approach. In fed-batch DAMP4 product titer increased 9-fold compared to batch, while maintaining 60% specific productivity. Under the fed-batch conditions, the final product titer of DAMP4 reached more than 7 g/L which is the highest titer of DAMP4 reported to date. To investigate production from sucrose, sucrose metabolism was engineered into BL21(DE3) using a simple plasmid approach. Using this strain, growth and DAMP4 production characteristics obtained from CDM supplemented with sucrose were similar to those obtained when culturing the parent strain on CDM supplemented with glucose.
Production of a model peptide was increased to several grams per liter using a CDM medium with either glucose or sucrose feedstock. It is hoped that this work will contribute cost reduction for production of designer peptide surfactants to facilitate their commercial application.
- Peptide production
- E. coli
Peptides are routinely produced by solid-phase chemistry for high-value, fine chemicals applications such as pharmaceuticals –. As fine chemicals, peptides are assumed to be expensive to produce . However, microbial cells are naturally competent for making and polymerizing amino acids and designer peptides can be recovered by simple cell lysis. Synthetic ‘designer’ peptides can be considered highly programmable polymers that can be precisely assembled from monomers (amino acids) and have applications as highly functional materials with innovative properties. Factors influencing the final cost of recombinant products include the price of feedstock, specific productivity and product titer, and downstream processing costs and efficiency .
Short Peptide Surfactants (SPS) are a class of industrial surfactants designed with self-assembly and stimuli-responsive properties , that could potentially replace traditional petrochemical surfactants such as those used as food additives, detergents and environmental applications –, if they could be produced at low cost ,. The model SPS, DAMP4, is the product of numerous studies ,–. Expression of this SPS as four tandem repeats of the functional unit  was found to increase yield to ~40% of the Total Cell Proteins (TCP) . Equally, simple thermal treatments and/or salting-out techniques have been developed to recover the product, greatly reducing downstream processing costs . Despite attempts to improve biological peptide production, by optimizing growth medium composition  and induction conditions , current product titers have not surpassed a few hundred mg/L .
Industrial production of low cost commodities in Chemically Defined Media (CDM) with simple sugars as carbon feedstock may lower specific productivity but it provides greater process control and increased process reproducibility , and it reduces peptide contamination  when compared to complex media alternatives. Typically, glucose would be used as the carbon feedstock, however, sucrose from sugarcane is an ideal feedstock for industrial microbial production as it is inexpensive to refine  and has impressive environmental credentials . Despite these advantages, sucrose is not widely used as a feedstock for E. coli as the majority of industrial E. coli strains do not naturally metabolize sucrose. But recent advances in the understanding of sucrose metabolism in E. coli and subsequent strain engineering have created strains that can grow on sucrose at the same rate as they do on glucose ; as well as strains that produce 1,4-BDO , carotenoids , or succinic acid . To date, however, no strain has been engineered to produce peptides or proteins from sucrose, nor has that production been scaled up to high cell density with sucrose as the sole carbon source in engineered E. coli.
In this study, E. coli BL21 was engineered to metabolize sucrose and used in the production of the SPS DAMP4. DAMP4 production was characterized on rich complex media as well as glucose and sucrose based minimal media in batch and fed-batch fermentation systems. To the best of our knowledge, this is the first report to describe production of a model SPS in high cell density cultures using an engineered strain to metabolize sucrose.
Batch bioreactor complex medium
DAMP4 production in complex media
Batch bioreactor CDM with glucose or sucrose substrates
DAMP4 production in a chemically defined minimal media (CDM) using glucose feedstock
The use of CDM in industrial processes can reduce media cost, maximize substrate conversion into product and minimize interference of media components with the purification of the peptidic product of interest. To investigate the effect of CDM on the production of DAMP4, the batch fermentations were repeated using CDM supplemented with glucose (CDMG) (Additional file 1: Figure S1). As expected, switching from rich complex media to CDM reduced growth rate and final biomass concentration. This reduction in CDM was attributed to the cells’ need to divert carbon from fuelling reactions and precursor generation to meet the requirements of complete anabolic metabolism ,. Following induction at 1 g/L DCW, biomass peaked at 2.5 g/L DCW, down from 4 g/L DCW observed for LBG cultures. Production of DAMP4 was also effected; total yield of DAMP4 was reduced from ~1 g/L in LBG to ~0.5 g/L in CDMG, corresponding to a maximum yield of ~36% DAMP4/TCP in ~4 h expression.
Engineering sucrose metabolism in E. coli BL21 (DE3)
As previously established, production of DAMP4 from sucrose would have several advantages over production from glucose, however, most E. coli production strains do not naturally metabolize sucrose. To allow production of DAMP4 from sucrose, the host strain E. coli BL21(DE3) pEDA was engineered to metabolize sucrose by co-transforming it with the plasmid p15aCSCx which encodes the cscAKB operon from E. coli W . Provision of sucrose in the media as the sole carbon source was sufficient for plasmid maintenance. Culturing the engineered strain in a bioreactor confirmed that growth rate and biomass yield in sucrose was unchanged when compared to the parent strain in glucose (data not shown). This is in stark contrast to previously published examples of sucrose engineering in E. coli in which strains were shown to have unstable sucrose utilization phenotypes, as observed in E. coli B  and W3110  or demonstrated a reduced growth rate on sucrose when compared to glucose as observed in engineered E. coli K-12 strains ,,.
Production of DAMP4 was also repeated using CDM supplemented with sucrose (CDMS) using 1 g/L DCW as the point of induction (Additional file 1: Figure S1). The production characteristics (growth rate, biomass and DAMP4 accumulation) on CDM supplemented with sucrose were similar to those obtained from cells cultured on CDM supplemented with glucose (Additional file 1: Figure S1, compare left and right panels).
Optimization of production – role of cell density at induction
Yields of recombinant DAMP4 obtained using either Sucrose or Glucose substrates and induced at DCW m during batch cultivation or induced at DCW i with F f feeding regimen for fed-batch cultivation
Induction point, Feeding rate
171.18 ± 6.37
6.7 ± 0.7
10.4 ± 0.8
126.44 ± 7.64
6.1 ± 0.4
8.6 ± 0.9
141.46 ± 10.75
5.4 ± 0.3
9.8 ± 1.6
114.94 ± 15.66
4.3 ± 0.2
7.1 ± 0.2
Rates of consumption/production for main cultivation parameters in Batch or Fed-batch cultivation (expressed as [mmol-C/gDCW*h] unless otherwise stated)
LB + glucose
48.3 ± 1.3
27.5 ± 3.6
23.5 ± 2.2
0.0 ± 0
23.2 ± 1.1
16.3 ± 2.8
15.9 ± 3.1
3.6 ± 0.3
2.6 ± 0.3
50.2 ± 0.9
24.2 ± 0.3
23.8 ± 2.1
0.6 ± 0.0
1.9 ± 0.1
0.0 ± 0.0
25.2 ± 0.6
8.9 ± 0.4
13.2 ± 0.5
1.9 ± 0.2
0.0 ± 0.0
2.2 ± 0.1
54.6 ± 0.6
24.3 ± 0.5
23.6 ± 0.1
1.9 ± 0.5
0.4 ± 0.1
0.0 ± 0.0
28.2 ± 0.4
10.0 ± 1.5
14.6 ± 0.3
2.9 ± 0.1
0.6 ± 0.1
2.1 ± 0.1
▪ Fed Batch
54.3 ± 0.8
23.3 ± 0.3
24.1 ± 1.4
0.6 ± 0.1
2.0 ± 0.4
0.0 ± 0.0
22.5 ± 0.9
9.8 ± 0.2
11.0 ± 0.6
0.0 ± 0.0
0.1 ± 0.0
0.0 ± 0.0
4.0 ± 0.2
1.2 ± 0.1
2.0 ± 0.3
0.1 ± 0.0
0.0 ± 0.0
0.4 ± 0.0
57.9 ± 1.5
25.1 ± 0.3
25.6 ± 1.1
0.8 ± 0.2
2.6 ± 0.2
0.0 ± 0.0
24.9 ± 0.6
11.1 ± 0.1
13.2 ± 0.2
0.0 ± 0.0
0.1 ± 0.0
0.0 ± 0.0
4.6 ± 0.5
1.3 ± 0.4
2.7 ± 0.6
0.1 ± 0.0
0.0 ± 0.0
0.4 ± 0.0
By-product formation directs valuable resources away from the production of the recombinant peptide of interest. During batch cultivation acetate accumulation was observed after induction, reaching ~1.2 g/L maximum (Figure 2), which is consistent with previous observations ,. The shift to acetate production following induction could be partly attributed to the over-representation of certain amino acids (namely Arginine and Methionine) in DAMP4. The amino acid composition of DAMP4 is such that up to 13 mol acetate could be formed per mol DAMP4 as by-product of the production of methionine and arginine. Specifically methionine biosynthesis from a cysteine precursor produced by the cysteine synthase complex (EC 220.127.116.11) results in the production of 1 mol acetate per mol of methionine. In the arginine biosynthesis, the formation of ornithine through the acetyl-ornithine deacetylase (EC 18.104.22.168) yields 1 mol acetate per mol of Arginine. Alternatively, acetate formation could be the product of additional ATP generation required to support recombinant protein formation , or due to an increased flux around the pyruvate node ,.
Cultivation and product formation on chemically defined medium fed-batch
Growth rate at induction can influence product accumulation (reviewed in ). In the case of DAMP4, maximum product formation was achieved when induction was performed with cells growing at μmax. Presented data clearly showed the dependence of product titer on feeding rate, which is known to influence cells’ growth rate and physiology , energy and precursors generation , plasmid stability , etc. and in turn it might affect protein accumulation . In addition, the high stress of high density cultures may significantly contribute to the decrease in specific productivity.
Maximum carbon yield and highest production rate of DAMP4
The performance of the two sugar substrates were compared using carbon moles, with the carbon balance for each condition closed to an average of 102.8 ± 5.3% (Table 2, and Additional file 2: Table S2). DAMP4 yield on batch cultures was ~6% for the whole process and a maximum of ~12% for the sole production phase on both substrates; on fed-batch processes, glucose cultures at fast feeding performed best reaching a product yield of more than 5% for the whole process and ~10% for the production phase (Table 1). DAMP4 accumulation rates varied considerably between batch and fed-batch cultures, owing to the different growth rate for the two-cultivation modes. Indeed, the highest observed DAMP4 production rate in batch cultures was ~2.4 mmol-CDAMP4/(gDCW*h), while in fed-batch this was ~0.4 mmol-CDAMP4/(gDCW*h) during production at fast feeding (Table 2). After induction growth rate decreased whereas CO2 and acetate production rates increased compared to un-induced growth. Overall, the cultivation process converted most of the substrates into CO2 (~65%) and biomass (~30%), with DAMP4 taking maximum ~6% of the substrate. HCDC on glucose had the lowest reduction in product formation compared to batch cultivations. The complete dataset for carbon distribution into products is available as additional material (Additional file 2: Table S1).
The substrate limited fed-batch cultivation, feeding carbon at constant rate, proved to be a simple and effective technique to grow cells to high density and to contain overflow metabolism as demonstrated by the absence of acetate accumulation during the feed phases prior to induction. E. coli BL21(DE3) grew up to ~50 g/L DCW in minimal medium fed only with carbon and nitrogen sources and MgSO4. Comparing batch cultivation (Gm, Sm) with fed-batch cultivation (Gf, Sf), final cell density and product titer increased ~8-fold and ~6-fold, respectively, with DAMP4/TCP decreasing of ~0.7-fold (Figures 2 and 3), but the DAMP4 production rate was only about 15% of that reported for the batch phase (Table 2). Growth rate decreased constantly as cell concentration rose during un-induced cultivation at constant feeding (Figure 3). Consistent with the observation that batch product formation rates were highest when cells were induced at μmax, the induction in fed-batch during fast feeding (growth rate higher) led to a higher accumulation of DAMP4 and process time was shorter than at slow feeding. This can be explained by previous observations that E. coli exhibits both a more efficient amino acid synthesis and charging of tRNAs  and a more efficient energy generation  during recombinant protein production at fast feeding. The undesired accumulation of acetate  in the fed-batch experiments was moderate. A maximum of around 4 g/L could be observed, which was also consistent with the batch data. This means that in the case of DAMP4 production with BL21(DE3), we did not reach the inhibitory concentration of 5 g/L reported previously . In some cases acetate remained below 1 g/L and most certainly, the ceasing of DAMP4 accumulation was not caused by acetate toxicity; indeed most acetate accumulated after peptide production stopped (Figure 3).
In this work we established the production of the short surfactant peptide DAMP4 on chemically defined medium, extended production to sucrose by re-engineering the existing production process to metabolize sucrose and increased product titer to several grams per liter of culture through the use of high cell density cultures (HCDC). Significantly, expression of DAMP4 was stable and product titer was similar on glucose or sucrose. Data showed that more than 6.5 g/L of the recombinant peptide could be produced from both glucose and sucrose. The production process reported in this work has model characteristics for the efficient production of other designed peptides.
Bacterial strains and plasmids
E. coli BL21(DE3) was the expression host. The peptide surfactant DAMP4 NH2-MD(PSMKQLADS-LHQLARQ-VSRLEHAD)4-COOH was expressed from the pET48b(+) (Merck Millipore, Kilsyth, Victoria, Australia) based vector pEDA . The plasmid was maintained using Kanamycin (Merck Millipore) at 50 μg/ml final concentration. Expression of DAMP4 was induced by the addition of IPTG (Merck Millipore) at 1 mM final concentration. Sucrose catabolism was conferred by plasmid p15aCSCx, carrying the cscAKB operon from E. coli W  expressed from a pACYC184  based vector. Selection was achieved using sucrose. Transformations were performed as described in . The resulting strains E. coli BL21(DE3) pEDA and E. coli BL21(DE3) pEDA,p15aCSCx were stored in 50% glycerol-R/2 solution at −80°C. DAMP4 gene was sequence-verified before and after cultivation.
Media and chemicals
All chemicals were of analytical grade and obtained from Sigma Aldrich (Castle Hill, NSW, Australia). Ultrapure water (18 MΩ/cm) was used. Tryptone, yeast extract and agar were obtained from Becton, Dickinson & Co., Sparks, MD, USA.
Complex medium: Lysogenic broth (LB)  with 20 g/L glucose (LBG) was the liquid complex medium. Solid medium contained 15 g/L agar. All media were sterilized by autoclaving, except for glucose solution that was filter sterilized and added separately.
Chemically defined minimal medium (CDM): R/2 was adjusted to pH 6.9 with KOH and supplemented with either sucrose (CDMS) or glucose (CDMG) as the sole carbon source at a final concentration of 20 g/L. CDM was filter sterilized with a 0.22 μm polyethersulfone membrane (Merck Millipore).
Determination of cell density
Cell growth was followed by optical density at 600nm (OD600) in a UV–VIS spectrophotometer (Libra S4, Cambridge, England). For LBG medium, blanks were performed against LBG medium in the same aqueous dilution as the sample. For CDM, water was used as blank. Dry cell weight was determined collecting 2 mL of culture medium in triplicate in a pre-weighted tube, which was centrifuged (3K30, Sigma Laborzentrifugen Gmbh, Osterode, Germany) at 13,500 × g, 4°C for 5 min, the cell pellet was then collected and washed with ice-cold water, re-pelleted, frozen and freeze-dried until constant weight was obtained.
All cultivations were performed at least in biological duplicates. Bioreactor experiments were carried out in parallel bioreactor system (DasGip, Juelich, Germany). The pH was maintained at 6.9 by addition of 25% NH4OH. Dissolved Oxygen (DO) was monitored by an external DO meter (Presens, Regensburg, Germany) and maintained at 70% of air saturation by automatic control of pure O2 enrichment. Temperature, stirring and gas flow were kept at 37°C, 800 rpm and 12 standard liters per hour (sL/h) using electronic mass flow control, respectively. Concentration of CO2 in the off-gas was monitored online using a gas analyzer (GA04, DasGip). Reactor volume, gas flow and CO2 concentrations were used to determine the CTR and hence the amount of CO2 (mmol-CO2) transferred during cultivation. Initial culture volume was 0.2 L, containing 0.1% v/v Antifoam C. Inocula for bioreactors were generated in shake flasks (250 mL baffled flasks in a Multitron orbital (2.5 cm) shaker (Infors, Noble Park North, VIC, Australia) at 200 rpm, 37°C and 50 mL culture volume), as described before  using the same medium as the respective main culture. Experimental data were used to calculate the cell density for induction to consume a given quantity of substrate using the formula DCWi = SStotal/(Yxs + Y’xs), where DCWi is the dry cell weight at the point of induction [g/L], SStotal is the total substrate concentration [g/L], Yxs and Y’xs are the amount of sugar needed per unit of biomass generated before and after induction, respectively [g/g]. Fed-batch cultivations started as a batch culture and constant feeding commenced at ~9g/L DCW, approximately 5 hours after culture start. The feeding regimen was 5.5 mL/h for fast feeding (feed rate = FF) and 4.6 mL/h for slow feeding (feed rate = FS); the feed consisted of carbon source (600g/L), MgSO4 (10g/L), (NH4)2SO4 (10g/L), kanamycin (50 μg/ml), Antifoam C (0.1% v/v) and water. Feed rate was calculated based on the desired cell density and growth rate at induction as reported in .
Quantification of substrates and products
Samples for extracellular metabolite analysis were collected at regular intervals during the entire process and samples for protein analysis were collected immediately prior to induction and at regular intervals afterwards. For each sample point, cells were harvested by centrifugation (13,500 × g, 4°C, 5 min). OD600 was recorded, the supernatant was transferred to a fresh tube and the cell pellet was washed with sterile H2O; both samples were kept at −80°C until further use. Prior to HPLC injection, extracellular metabolite samples were thawed on ice and filtered with a 3 KDa molecular weight cut-off filter (Merck Millipore) according to manufacturer’s directions. HPLC analysis was performed as described previously . The substrates and products quantified by HPLC were formate, acetate, and glucose, fructose and sucrose.
DAMP4 was quantified using SDS-PAGE. For this, cell pellets were resuspended in 10% solution BugBuster 10X reagent (Merck Millipore) and sterile H2O, such that the total protein concentration of the final mixture was suitable for loading on the gels. An aliquot was withdrawn and mixed (1:2) with Laemmli Sample Buffer (Biorad, Gladesville, NSW, Australia) and incubated (12 min, 80°C). Identical protein amounts (1–0.1 μg/well) were loaded onto precast 12% NuPAGE SDS-PAGE gels (Life Technologies, Mulgrave, Victoria, Australia) and run for 65 min at 200V in MES buffer (Life Technologies). Gels were rinsed 3 times with H2O, stained with Coomassie Blue (Life Technologies) for 30 min, destained in H2O overnight, imaged and analyzed with Image Lab 4.0 (Biorad, Gladesville, NSW, Australia) using 3 mm background correction sphere. Quantification was then achieved by densitometry using a standard curve (0.75, 0.5, 0.25, 0.1 μg/well) of purified DAMP4 (purity > 90% by HPLC) included on each gel and by determining the abundance of recombinant DAMP4 on total cell proteins and expressed as % of total cell protein (D4/TCP). About ~92 ± 10% of the spiked pure peptide on a negative control could be recovered. Total cell protein (TCP) was determined using Bradford assay (Thermo Fisher Scientific Australia, Scoresby Victoria, Australia). DAMP4 was not detected in supernatant fractions.
We would like to thank Dr. Linda Lua (Protein Expression Facility, University of Queensland, St. Lucia, Australia) for kindly providing vector pEDA . We also want to thank Prof. Anton Middelberg for the supply of DAMP4 standard, Ms Sarah Bydder for her help with the strain construction and Dr. Manuel Plan (Metabolomics Australia, University of Queensland, St. Lucia, Australia) for his help with analytics. Jens O. Krömer was financially supported by the Australian Research Council (DE120101549).
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