- Open Access
Endotoxin-free purification for the isolation of Bovine Viral Diarrhoea Virus E2 protein from insoluble inclusion body aggregates
- Antonino S Cavallaro†1,
- Donna Mahony†1,
- Margaret Commins1,
- Timothy J Mahony2 and
- Neena Mitter2, 3Email author
© Cavallaro et al; licensee BioMed Central Ltd. 2011
- Received: 3 April 2011
- Accepted: 26 July 2011
- Published: 26 July 2011
Protein expression in Escherichia coli may result in the recombinant protein being expressed as insoluble inclusion bodies. In addition, proteins purified from E. coli contain endotoxins which need to be removed for in vivo applications. The structural protein, E2, from Bovine Viral Diarrhoea Virus (BVDV) is a major immunogenic determinant, and is an ideal candidate as a subunit vaccine. The E2 protein contains 17 cysteine residues creating difficulties in E. coli expression. In this report we outline a procedure for successfully producing soluble and endotoxin-free BVDV E2 protein from inclusion bodies (IB).
The expression of a truncated form of BVDV-E2 protein (E2-T1) in E. coli resulted in predominantly aggregated insoluble IB. Solubilisation of E2-T1 with high purity and stability from IB aggregates was achieved using a strong reducing buffer containing 100 mM Dithiothreitol. Refolding by dialysis into 50 mM Tris (pH 7.0) containing 0.2% Igepal CA630 resulted in a soluble but aggregated protein solution. The novel application of a two-phase extraction of inclusion body preparations with Triton X-114 reduced endotoxin in solubilised E2-T1 to levels suitable for in vivo use without affecting protein yields. Dynamic light scattering analyses showed 37.5% of the protein was monomeric, the remaining comprised of soluble aggregates. Mice immunised with E2-T1 developed a high titre antibody response by ELISA. Western hybridisation analysis showed E2-T1 was recognised by sera from immunised mice and also by several BVDV-E2 polyclonal and monoclonal antibodies.
We have developed a procedure using E. coli to produce soluble E2-T1 protein from IB, and due to their insoluble nature we utilised a novel approach using Triton X-114 to efficiently remove endotoxin. The resultant protein is immunogenic and detectable by BVDV-E2 specific antibodies indicating its usefulness for diagnostic applications and as a subunit vaccine. The optimised E. coli expression system for E2-T1 combined with methodologies for solubilisation, refolding and integrated endotoxin removal presented in this study should prove useful for other vaccine applications.
- Inclusion Body
- Bovine Viral Diarrhoea Virus
- Disulphide Bond
- Subunit Vaccine
- Japanese Encephalitis Virus
Bovine viral diarrhoea virus (BVDV) infection of cattle is linked to economically important diseases with losses in the USA being estimated to US$10-40 million per million calves  and US$6 million per million calves in the UK . BVDV is a member of the Pestivirus genus within the Flavivirus family. The BVDV genome is a positive sense RNA molecule with one open reading frame (ORF) encoding for a polyprotein which is cleaved into the structural and non-structural proteins . Of the structural proteins, the surface glycoprotein, E2 is a major immunogenic determinant and is involved in virus neutralisation . E2 is therefore an ideal candidate for use in subunit vaccines [5, 6].
E2 contains 17 cysteine residues which form both intramolecular disulphide bonds and intermolecular disulphide bonds resulting in dimers of E2-E2 and E2-E1 . For a protein with high disulphide bond formation, recombinant protein expression is best attempted in mammalian and insect cell systems . Expression of E2 has been documented in mammalian [5, 9] as well as insect cell lines [5, 10, 11] and an insect larval system . Mammalian and insect cell line expression of proteins have the advantage of producing proteins with correct conformation and post-translational modifications such as glycosylation, but generally yields are lower than Escherichia coli systems. However, the low costs required for veterinary vaccine applications preclude the use of more expensive protein expression systems such as mammalian and insect cell systems . The use of E. coli based expression systems is hindered by the fact that although the recombinant proteins are generally expressed at high yields the resulting proteins are often insoluble and lack post-translational modifications . Expression of glycosylated proteins in E. coli has been previously reported, Chia et al.  demonstrated the successful generation of neutralising antibodies to the envelope protein (E) of Japanese Encephalitis Virus (JEV), also a member of the Flavivirus family. Das et al.  demonstrated monoclonal antibodies generated against E. coli expressed Ebola virus antigen recognised the glycosylated antigen expressed in mammalian cells.
Expression of recombinant proteins in E. coli often leads to insoluble aggregates known as IB . Though, usually seen as an undesirable effect, recent research has shed light on advantages of IB formation . Furthermore as IB aggregates are observed due to intermolecular interactions among a single type of protein, the formation of IB can aid in the purification and isolation of the expressed protein . IB aggregates are common in proteins containing disulphide bonds (such as E2), as the reducing environment of the bacterial cytosol inhibits the formation of disulphide bonds [8, 19]. IB solubilisation is generally achieved by the use of chaotropic agents, such as urea and guanidine salts, and/or detergents and reducing agents. Refolding of the protein can be achieved by dilution or dialysis into suitable buffers that may contain detergents, oxidising or reducing agents and other additives to maintain solubility and to facilitate correct folding of the protein [19, 20].
A potential drawback from the production of recombinant proteins in E. coli is contamination with endotoxins. Endotoxins are a major component of gram negative bacterial cell walls and are liberated during extraction of proteins . Endotoxins are heat stable lipopolysaccharides with monomer molecular weights ranging from 10 to 20 kDa and form highly stable aggregates . Mammalian exposure to endotoxins can induce several undesirable physiological effects such as fever, leukocytosis, hypoferremia, platelet aggregation, thrombocytopenia and coagulapathies . Common methods employed for the removal of endotoxins from protein purifications include ultrafiltration, adsorption techniques, affinity chromatography and Triton X-114 two-phase extraction [21, 23]. Two-phase extraction with Triton X-114 showed 98-99% reduction of endotoxin levels for the soluble proteins cardiac troponin I, myoglobin and creatin kinase with a protein recovery of > 90% . Aida and Pabst  demonstrated a 1000 fold reduction of endotoxin for the soluble proteins catalase, cytochrome c, and bovine serum albumin using this method with a protein loss of 2% for cytochrome c.
In this study, we report the expression and purification of a truncated form of the BVDV E2 protein (E2-T1) from IB aggregates and optimised solubilisation conditions for this protein. We also describe a novel process for the removal of endotoxins from IB aggregates using Triton X-114 phase-partitioning to maximise E2-T1 yields. The suitability of this E2-T1 protein for small animal vaccination in mice is also demonstrated.
Cloning and Expression
A truncated version of the E2 ORF frame was produced using PCR to remove the 3' region of the ORF which encodes for the membrane binding domain. The resultant 1040 bp PCR product was ligated into pET-SUMO expression vector.
Amino Acid composition of E2-T1
Purification and Refolding
Purification of E2-T1 from the soluble protein fraction was attempted using TALON resin. A step gradient of imidazole (50, 80, 100 and 150 mM) was used to determine the optimum elution profile. At 150 mM imidazole, E2-T1 was the major species eluted from the column. This eluted protein was of high purity but of low yield (10 ng/μL).
The majority of the E2-T1 protein was present in the insoluble fraction (Figure 1A, B). Using BugBuster™ it was possible to prepare soluble, high purity E2-T1 from the IB. E2-T1 protein was successfully dissolved in a DTT-SDS buffer (50 mM Tris (pH 6.8), 100 mM DTT, 1% SDS, 10% Glycerol). Titration of DTT concentrations using 5, 10 and 20 mM revealed a degree of solubility at all DTT concentrations; however, only at 100 mM DTT was the entire fraction of E2-T1 protein consistently solubilised (data not shown).
Refolding of E2-T1 protein was achieved by dialysis in 50 mM Tris (pH 7.0), 0.2% Igepal at room temperature. The resultant protein had high purity (Figure 1A, lane 6) with an average yield of 1-2 mg protein/litre of bacterial culture and was highly stable. E2-T1 stored at -20°C showed no degradation after more than 12 months and was resistant to degradation at room temperature for 7 days (data not shown).
Initial attempts to refold E2-T1 in 50 mM phosphate buffer (pH 6.0) and PBS (pH 7.2) were unsuccessful, as the protein formed insoluble aggregates, the addition of Igepal CA630 to 0.2% failed to improve protein solubility in these buffers. However, E2-T1 protein remained soluble in 50 mM Tris (pH 8.0), 0.2% Igepal CA630 and 50 mM Tris (pH 7.0), although in the absence of Igepal CA630, E2-T1 showed a much higher level of polydispersity (PdI: 0.931 ± 0.075).
Purified protein concentrations and endotoxin levels
The terminal bleed serum from one animal with the highest ELISA response was used in Western hybridisation analyses to E2-T1. Preimmune sera from this animal showed no reactivity at 1:200 and 1:4000 dilution (Data not shown). Specific detection of E2 protein was detected at high titre (1:64000) with mouse serum (Figure 5B). Non-specific bands were also observed, although E2-T1 was the dominant reactive species. The non-specific bands were not detectable by the preimmune sera.
The advantages of IB in terms of biological activity and facilitating protein purification have been highlighted in recent publications (15, 16). This study describes a procedure for the expression and solubilisation of a highly purified viral antigen derivative, E2-T1 from IB. The methodology includes the efficient removal of endotoxins to allow for potential in vivo applications.
In vivo refolding studies of purified E2 have shown that intramolecular disulphide bonds form rapidly within 2.5 minutes and intermolecular disulfide bonds result in formation of E2 dimers . Since disulphide bonds are inefficiently formed in the reducing environment of the E. coli cytosol  and native E2 rapidly forms intramolecular disulphide bonds, misfolding of E2-T1 is likely to form an insoluble protein. Also, formation of intermolecular disulphide bonds between E2-T1 in the E. coli cytosol would lead to the formation of aggregates resulting in IB. In our study consistent and reproducible solubilisation of E2-T1 was only achievable using a highly reducing buffer containing 100 mM DTT. At lower DTT concentrations (20 to 5 mM), the percent solubility of E2-T1 decreased, indicating strong disulphide bond formation. The inclusion of DTT as a reducing agent in the re-suspension buffer would disrupt incorrectly formed disulphide bonds, and then during dialysis into DTT-free buffer, the disulphide bonds could reform in a conformation that is more suitable for soluble protein.
Although refolding of E2-T1 was successful in Tris based buffers, the resultant protein formed soluble aggregates as indicated by a PdI of 0.931. The soluble aggregation could be due in part to the same intermolecular disulphide bond formation reported for native E2. The addition of the detergent Igepal CA630 (0.2%) to Tris based buffers reduced aggregation (PdI 0.528), indicating some aggregation may be due to weaker intermolecular interactions such as ionic and/or hydrogen bonds. Under non-reducing electrophoresis conditions (Figure 2B), E2-T1 shows 2 dominant bands corresponding to monomeric and dimeric forms. This corresponds to the dimeric bonds between dimers arising from disulphide bond formation and other soluble aggregation is due to weaker intermolecular interactions. Addition of Igepal CA360 to PBS (pH 7.2) could not reverse the formation of aggregates indicating that the presence of Tris may be critical for maintaining E2-T1 solubility. The fact that a highly reducing buffer (100 mM DTT) was required to solubilise E2-T1 IB and the addition of Igepal CA360 could not completely overcome aggregation, lends evidence to strong disulphide bond formation.
Endotoxin levels lower then 3 EU/mL of E. coli derived proteins have been reported to be safe, causing no adverse reactions in animal trials [26, 27]. However, in our case the E2-T1 protein purified from E. coli resulted in high endotoxin levels between 5.29 - 199.31 EU/mL. This was considered unsuitable for testing E2-T1 as a component of a veterinary vaccine due to the risk of adverse immunological reactions. Commercially available techniques for endotoxin removal typically employ affinity columns and require buffer changes for washing and elution of the protein. Attempts to use ion exchange chromatography were discontinued due to consistently low recovery of E2-T1.
We introduced a significantly innovative step for endotoxin removal from the E. coli IB by adding Triton X-114 in the E2-T1 expression and purification protocol prior to solubilisation and recovery of the target protein. Phase separation with Triton X-114 resulted in up to 600 fold reduction in the endotoxin levels of the E2-T1 preparations (Table 2). Importantly, using this method resulted in no detectable E2-T1 loss (Figure 3), as the protein remained insoluble within the IB. This approach could be generally applicable for the efficient removal of endotoxins from other proteins contained within IB preparations, by maintaining the IB in a buffer incompatible with the solubilisation of the target protein, while still facilitating endotoxin removal with Triton X-114.
We have shown that E2-T1 protein produced in E. coli was recognised by antibodies raised in goat and sheep against whole BVDV and also by various BVDV-specific monoclonal antibodies (Figure 4) indicating the usefulness of E2-T1 for diagnostic applications such as monitoring the serological status of animals which are the natural host of BVDV. Furthermore an ELISA done using E2-T1 against 5 BVDV infected cattle sera samples with known serum neutralisation titres showed that E2-T1 is recognised by cattle sera at a comparable level to the commercial positive control sera (data not shown).
One monoclonal antibody, mAb-D89, did not recognise E2-T1, which could be due to its binding to either a conformational E2 epitope or an epitope that is dependent on post-translational modification of E2 such as glycosylation. As the binding capacity of mAb-D89 was only assessed under denaturing and reducing conditions this could have caused the loss of the mAb-D89 epitope from the renatured E2-T1. It remains to be determined how the potential loss of spatial and other non-linear epitopes of native E2 would affect the efficaciousness of any vaccine formulations containing E2-T1.
Immunisation of mice with bacterially derived E2-T1 protein resulted in an excellent immune response, confirmed both by ELISA assay and Western blot hybridisation. Western blot analysis with mouse sera collected after three immunisations with E2-T1 resulted in very strong detection of E2 protein with significant bands readily detectable at a 1:64000 dilution. The predominant lower molecular weight band (approximately 45 kDa) observed by Western hybridisation (Figure 5B) may be due to the polyclonal nature of the antibodies and are not present when probed with pre-immune sera.
The results of this study demonstrate that the bacterially derived E2-T1 protein solubilised from IB can induce an excellent humoral response in small animals and could potentially be used as a subunit vaccine. The next step will be to determine if E2-T1 can elicite similar responses in large animals such as sheep or cattle when evaluated as a potential vaccine antigen.
The development of cost effective veterinary vaccines and diagnostics requires the use of efficient methods that enable the production of large quantities of immunogenic and non-toxic proteins. Using an E. coli system and exploiting the formation of IB, we were able to produce a highly pure, stable and endotoxin-free E2-T1 protein. It was highly immunogenic in mice and was recognised by BVDV-E2 specific antibodies raised to native E2 in BVDV. We have developed a procedure for solubilising and refolding E2-T1 as well as the removal of endotoxin by Triton X-114 two-phase extraction which offers an elegant solution for the production of other proteins intended for diagnostic uses and in vivo uses such as subunit vaccines or therapeutics.
Cloning of E2-T1 into pET-SUMO bacterial expression vector
The E2 gene was amplified from a plasmid containing BVDV isolate MD74 which has been identified as a type-1 isolate . Twenty μL of Qiagen (Venlo, The Netherlands) PCR master mix was used with primers at a final concentration of 0.5 μM. The forward primer nanoE2-F sequence was 5'-ATGGTGGATCCGTGCAAGCCT-3' and the reverse primer nanoE2-Rtrunc1 sequence was 5'-CTAAGACTCGGCGAAGTAGTCCCGG-3'. PCR cycling conditions comprised an initial incubation at 95°C for 5 minutes, followed by 35 cycles at 94°C for 30 seconds, 60°C for 30 seconds and 72°C for 90 seconds. The resultant 1040 bp product was ligated into the pET-SUMO vector (Invitrogen, Carlsbad, USA). The ligation products were subsequently transformed into electrocompetent E. coli strain DH10B (Invitrogen). Positive clones were confirmed by sequencing (AGRF, Brisbane, Australia) and transformed into E. coli strain BL21 (DE3, Invitrogen) cells for protein expression.
Large-scale expression and purification of E2-trunc1 protein
An overnight culture of E. coli BL21 (DE3) containing pET-SUMO-E2-T1 was used to inoculate four 250 mL cultures of LB Miller broth (Amresco, Solon, USA) containing 50 mg/L Kanamycin-sulphate (Amresco). These cultures were grown at 37°C to an OD600 of 0.4 to 0.6, then induced with 1 mM IPTG and grown for a further 2 hours. The bacterial pellet was collected by centrifugation at 3,800 g, at 4°C for 15 minutes in 4 × 250 mL centrifuge tubes. Total protein was extracted by resuspending each bacterial pellet in 50 mL E. coli lysis buffer (50 mM KPO4 phosphate (pH 7.8), 400 mM NaCl, 100 mM KCl, 10% glycerol, 0.5% Triton X-100, 10 mM Imidazole), with the addition of 12.5 mg Lysozyme and 750 units of Benzonase nuclease (Novagen-Merck, Darmstadt, Germany). The bacterial suspensions were incubated in lysis buffer for 20 minutes with gentle shaking. The samples were frozen in liquid nitrogen, and thawed at 42°C three times. The resultant solution was centrifuged at 37,000 g at 4°C for 15 minutes. The insoluble protein fraction (containing IB aggregates) and the supernatant (containing the soluble protein fraction) were stored at -20°C until required.
Purification of soluble E2-T1
E2-T1 protein was purified from the soluble fraction by affinity chromatography using TALON (Clontech, Mountain View, USA) resin following manufacturer's instruction. Bound protein was eluted from the resin using TALON elution buffer with a step gradient of 50 mM, 80 mM, 100 mM and 150 mM imidazole, collecting ten 500 μL fractions/step. Fractions were analysed by SDS-PAGE.
Purification of inclusion body aggregates of E2-T1
The insoluble protein fraction (including E2-T1) was recovered from the IB using BugBuster™ Master Mix (Novagen-Merck) as follows. IB pellets (equivalent to 160 mL bacterial culture) were resuspended in 2.5 mL BugBuster™ and vortexed for 2 minutes. Following the addition of 15 mL of 1:10 diluted BugBuster™ and further vortexing for 1 minute, the resuspended IB pellets were centrifuged at 5000 g at 4°C for 15 minutes. Three further washes of 25 mL 1:10 diluted BugBuster™ were performed with vortexing and centrifugation steps as above. Following the final wash step, the pellets were resuspended in 1 mL 1:10 diluted BugBuster™, transferred into 1.5 mL tubes and centrifuged at 16,200 g at 4°C for 15 minutes. The supernatant was removed and the IB pellets were stored at -20°C without any detectable protein degradation.
All reagents were prepared in endotoxin-free water (< 0.001 EU/mL, MO BIO Laboratories, Carlsbad, USA). Triton X-114 exhibits a cloud point at 22°C, above this temperature micelles aggregate forming a new phase with very low water content. Endotoxin remains in the detergent phase . Purified IB pellets were resuspended in 1 mL of PBS (137 mM NaCl, 2.7 mM KCl, 10 mM Phosphate buffer (pH 7.2), Amresco), and vortexed for 1 minute to disperse the insoluble protein. Dispersed protein solutions were mixed with 1% (v/v) of Triton X-114 by vigorous vortexing for 1 minute. Samples were incubated on ice for 5 minutes, vortexed and subsequently incubated at 56°C for 1 minute to allow phase separation. After centrifugation at 16,200 g at room temperature for 7 seconds in a microfuge the 3 phases (aqueous, oil and pellet) were recovered into separate tubes and analysed by SDS-PAGE electrophoresis.
To determine the level of endotoxin in the protein samples, endotoxin assays were performed by using the Limulus Amebocyte Lysate (LAL) assay by AMS Laboratories (Sydney, Australia).
Solubilisation of E2-T1
Protein pellets from the IB preparations were dissolved in 50 mM Tris (pH 6.8), 100 mM DTT, 1% SDS, 10% Glycerol, vortexed at low speed for 2 minutes and incubated at 37°C for 20 minutes. The resulting solubilised protein was dialysed at room temperature, with 3 buffer changes over 24 hours against 50 mM Tris (pH 7.0), 0.2% Igepal CA630 (Sigma-Aldrich). Following dialysis protein integrity was determined by SDS-PAGE analysis and protein yield determined by colourimetric assay (BioRad DC Kit, Hercules, USA). Other dialysis buffers evaluated in this study were: 50 mM Tris, (pH 7.0); 50 mM Tris (pH 8.0), 0.2% Igepal CA630; PBS (pH 7.2); PBS (pH 7.2), Igepal CA630; 50 mM phosphate buffer (pH 6.0).
SDS-PAGE analysis was performed using Invitrogen's XCell SureLock® Mini-Cell precast system with NuPAGE 10% BIS-Tris gels according to manufacturer instructions. Size estimations were determined against SeeBlue® Plus2 (Invitrogen) or Precision Plus Protein Kaleidoscope Standards (BioRad) pre-stained standards. The resolved proteins were visualised by staining in 50% methanol, 10% acetic acid, 0.25% Coomassie Blue R250 for 30 minutes, followed by destaining in 30% methanol, 10% acetic acid for 10 minutes three times.
Western Hybridisation Analysis
Following SDS-PAGE electrophoresis the resolved polypeptides were transferred to Hybond C nitrocellulose membrane (GE Healthcare, Buckinghamshire, United Kingdom) using Invitrogen XCell II™ Blot Module Kit according to manufacturer's instructions. All antibodies were diluted in BLOTTO (PBS (Amresco), 0.1% Tween 20, 1% skim milk). E2 specific monoclonal antibodies D89 , mAb-157 and mAb-348  and polyclonal goat anti-BVDV (VMRD, Pullman, USA). The pestivirus genus specific monoclonal 4-9D4 was kindly provided by Dr Linfa Wang . E2 specific monoclonal antibodies were used at 1:100 dilution. An anti-E2 sheep sera 804 was produced in vaccinated sheep after intramuscular injection of BVDV E2 and diluted to 1:500. Monoclonal 6× His antibodies (Clontech) were used at 1:15,000. Anti mouse immunoglobulin G HRP conjugate (Chemicon, Millipore, Billerica, Massachusetts, USA) and anti sheep/goat immunoglobulin HRP conjugate (Sigma) were used at 1:2,000 and 1:10,000 respectively. Detection was carried out using an ECL detection kit (GE Healthcare).
C57BL/6J mice were purchased from and housed in the Biological Resource Facility, The University of Queensland, Brisbane, Australia under specific pathogen free conditions. Female mice were housed in HEPA-filtered cages with 4 animals per cage in an environmentally controlled area with a cycle of 12 hours of light and 12 hours of darkness. Food and water were given ad libitum. All studies were conducted with 8 week old mice at the time of first injection. All procedures were approved by The University of Queensland Ethics Committee.
Immunisation of mice with E2-T1
Pre-immunisation blood samples of were collected by retro-orbital bleed using heparin coated hematocrit tubes (Hirschmann Laborgeräte Heilbronn, Germany). Pre-immunisation blood samples collected prior to the first immunisation were referred to as the preimmune samples. Blood samples collected 2 weeks after the third immunisation was referred to as terminal bleed.
All doses of E2-T1 were prepared in sterile conditions in a certified biological safety cabinet using sterile reagents, equipment and aseptic technique. The adjuvant QuilA (Superfos Biosector, Vedback, Denmark) was resuspended at 2 mg/mL in sterile injectable water (Pfizer, Brooklyn, USA).
Dose volumes were adjusted to 500 μL using 0.9% saline (Pfizer). 50 μg E2-T1 together with 10 μg QuilA, were administered in a final volume of 100 μL subcutaneously at the tail base using a sterile 27 gauge needle (Terumo, Tokyo, Japan). Three injections were administered at 2 week intervals and mice were sacrificed 14 days after the final immunisation. Animals were closely monitored throughout the study. All the animals remained in good health for the duration of the study with no visible deleterious health effects.
Humoral antibody responses
ELISA assays for the detection of E2-T1-specific antibodies were performed by coating microtitre plates (96 well, Nunc, Maxisorb, Roskilde, Denmark) with
50 μL E2-T1 antigen solution (2 ng/μL in PBS) overnight at room temperature. Antigen solution was removed from the plates which were then washed once with 1× PBS-T (1× PBS, 0.1% Tween: Sigma-Aldrich) and blocked with 200 μL per well of PBS containing 5% BSA (Sigma-Aldrich), 5% skim milk (Fonterra, Auckland, New Zealand) for 1 hour with gentle shaking at room temperature. Plates were washed three times in 200 μL 1× PBS-T as described above.
Mouse sera samples were diluted from 1:100 to 1:6400 and 50 μL of diluted sera was added to plates then incubated for 2 hours at room temperature. To detect mouse antibodies HRP conjugated polyclonal sheep anti-mouse IgG antibodies (100 μL of 1:10000 dilution in PBS (pH 7.2), Chemicon Australia, Melbourne, Vic, Australia) was added per well and incubated for 1 hour at RT with gentle shaking. Plates were washed three times in 200 μL 1× PBS-T and 100 μL of TMB substrate (Sigma-Aldrich) was added to each well. After 15 minutes at RT 100 μL of 1 N HCl was added to each well to stop the chromogenic reaction. Plates were read at 450 nm within 10 minutes.
Concentrating of E2-T1/Buffer Change
Protein concentration was increased by using 30 kDa Vivaspin 2 centrifugal filters (Millipore). Briefly, up to 2 mL of protein solution was added to the upper chamber and centrifuged (4000 g, 4°C) until the volume was reduced to the required amount. These columns were also used to perform buffer changes. After concentration of samples, the target buffer was replenished to the original volume.
Dynamic light scattering analysis
Size and polydispersity data were determined by dynamic light scattering (DLS) using a Malvern Instruments Zetasizer Nano (Worcestershire, UK.). E2-T1 solution (1 mL) was placed in a clear disposable zeta cell (DTS1060C, Malvern Instruments). Analysis was performed using the size standard operating procedure (SOP) for which the following parameters were use: material set to protein, dispersant set to water, taking 5 - 6 independent measurements of 30 runs each. The size and polydispersity index for samples were the average of all measurements. Analysis of the data was carried out by Malvern Zetasizer software.
Physical properties of E2-T1
Physical data was obtained using ProtParam, last accessed 3 March 2011 at http://au.expasy.org/tools/protparam.html.
Use of the Zetasizer at the Australian Research Council Centre of Excellence for Functional Nanomaterials is gratefully acknowledged. We also acknowledge the assistance of the Biological Resource Facility at the Australian Institute for Bioengineering & Nanotechnology at The University of Queensland for the animal care. We would like to thank Dr Linfa Wang for the gift of the monoclonal antibody 9-4D4. This work was funded by the Queensland Government through the Department of Employment, Economic Development and Innovation Reinvestment Fund.
- Mattiasson B, Adlercreutz P: Perfluorochemicals in biotechnology. Trends in Biotechnol. 1987, 5: 250-254. 10.1016/0167-7799(87)90101-6.View ArticleGoogle Scholar
- Lowe KC: Perfluorochemical respiratory gas carriers: benefits to cell culture systems. J Fluorine Chem. 2002, 118: 19-26. 10.1016/S0022-1139(02)00200-2.View ArticleGoogle Scholar
- Riess JG: Perfluorocarbon-based Oxygen Delivery. Artificial Cells, Blood Substitutes and Biotechnol. 2006, 34: 567-580. 10.1080/10731190600973824.View ArticleGoogle Scholar
- Lowe KC: Fluorinated blood substitutes and oxygen carriers. J Fluorine Chem. 2001, 109: 59-65. 10.1016/S0022-1139(01)00374-8.View ArticleGoogle Scholar
- Krafft MP: Fluorocarbons and fluorinated amphiphiles in drug delivery and biomedical research. Adv Drug Deliv Rev. 2001, 47: 209-228. 10.1016/S0169-409X(01)00107-7.View ArticleGoogle Scholar
- King AT, Mulligan BJ, Lowe KC: Perfluorochemicals and cell culture. Biotechnology. 1989, 7: 1037-1042.Google Scholar
- Riess JG: Oxygen carriers ('Blood substitutes') - Raison d'Etre, chemistry, and some physiology. Chemical Reviews. 2001, 101: 2797-2919. 10.1021/cr970143c.View ArticleGoogle Scholar
- Shiba Y, Ohshima T, Sato M: Growth and morphology of anchorage-dependent animal cells in a liquid/liquid interface system. Biotechnol Bioeng. 1998, 57: 583-589. 10.1002/(SICI)1097-0290(19980305)57:5<583::AID-BIT10>3.0.CO;2-D.View ArticleGoogle Scholar
- Rappaport C: Progress in concept and practice of growing anchorage-dependent mammalian cells in three dimension. In Vitro Cell Dev Biol Anim. 2003, 39: 187-192. 10.1290/1543-706X(2003)039<0187:RICAPO>2.0.CO;2.View ArticleGoogle Scholar
- Pilarek M, Szewczyk KW: Effects of perfluorinated oxygen carrier application in yeast, fungi and plant cell suspension cultures. Biochem Engin J. 2008, 41: 38-42. 10.1016/j.bej.2008.03.004.View ArticleGoogle Scholar
- Damiano D, Wang SS: Novel use of perfluorocarbon for supplying oxygen to aerobic submerged cultures. Biotechnol Lett. 1985, 7: 81-86. 10.1007/BF01026673.View ArticleGoogle Scholar
- Ju LK, Lee JF, Armiger WB: Enhancing oxygen transfer in bioreactors by perfluorocarbon emulsions. Biotechnol Progress. 1991, 7: 323-329. 10.1021/bp00010a006.View ArticleGoogle Scholar
- Krause M, Ukkonen K, Haataja T, Ruottinen M, Glumoff T, Neubauer A, Neubauer P, Vasala A: A novel fed-batch based cultivation method provides high cell-density and improves yield of soluble recombinant proteins in shaken cultures. Microb Cell Fact. 2010, 9: 11-10.1186/1475-2859-9-11.View ArticleGoogle Scholar
- Panula-Perälä J, Siurkus J, Vasala A, Wilmanowski R, Casteleijn MG, Neubauer P: Enzyme controlled glucose auto-delivery for high cell density cultivations in microplates and shake flasks. Microb Cell Fact. 2008, 7: 31-10.1186/1475-2859-7-31.View ArticleGoogle Scholar
- Glazyrina J, Materne EM, Dreher T, Storm D, Junne S, Adams T, Greller G, Neubauer P: High cell density cultivation and recombinant protein production with Escherichia coli in a rocking-motion-type bioreactor. Microb Cell Fact. 2010, 9: 42-10.1186/1475-2859-9-42.View ArticleGoogle Scholar
- Tegel H, Yderland L, Bostrom T, Eriksson C, Ukkonen K, Vasala A, Neubauer P, Ottosson J, Hober S: Parallel production and verification of protein products using a novel high-throughput screening method. Biotechnol J. 2011Google Scholar
- Weuster-Botz D: Parallel reactor systems for bioprocess development. Adv Biochem Eng Biotechnol. 2005, 92: 125-143.Google Scholar
- Betts JI, Doig SD, Baganz F: Characterization and application of a miniature 10 mL stirred-tank bioreactor, showing scale-down equivalence with a conventional 7 L reactor. Biotechnol Progr. 2006, 22: 681-688. 10.1021/bp050369y.View ArticleGoogle Scholar
- Schapper D, Alam MNHZ, Szita N, Lantz AE, Gernaey KV: Application of microbioreactors in fermentation process development: a review. Anal Bioanal Chem. 2009, 395: 679-695. 10.1007/s00216-009-2955-x.View ArticleGoogle Scholar
- Neubauer P, Junne S: Scale-down simulators for metabolic analysis of large-scale bioprocesses. Curr Opin Biotechnol. 2010, 21: 114-121. 10.1016/j.copbio.2010.02.001.View ArticleGoogle Scholar
- Siurkus J, Panula-Perälä J, Horn U, Kraft M, Rimseliene R, Neubauer P: Novel approach of high cell density recombinant bioprocess development: optimisation and scale-up from microliter to pilot scales while maintaining the fed-batch cultivation mode of E. coli cultures. Microb Cell Fact. 2010, 9: 35-10.1186/1475-2859-9-35.View ArticleGoogle Scholar
- Hermann R, Lehmann M, Büchs J: Characterization of gas-liquid mass transfer phenomena in microtiter plates. Biotechnol Bioeng. 2003, 81: 178-186. 10.1002/bit.10456.View ArticleGoogle Scholar
- Kensy F, Zimmermann HF, Knabben I, Anderlei T, Trauthwein H, Dingerdissen U, Büchs J: Oxygen transfer phenomena in 48-well microtiter plates: determination by optical monitoring of sulfite oxidation and verification by real-time measurement during microbial growth. Biotechnol Bioeng. 2005, 89: 698-708. 10.1002/bit.20373.View ArticleGoogle Scholar
- Neubauer P, Lin HY, Mathiszik B: Metabolic load of recombinant protein production: inhibition of cellular capacities for glucose uptake and respiration after induction of a heterologous gene in Escherichia coli. Biotechnol Bioeng. 2003, 83: 53-64. 10.1002/bit.10645.View ArticleGoogle Scholar
- Farr SB, Touati D, Kogoma T: Effects of oxygen stress on membrane functions in Escherichia coli: role of HPI catalase. J Bacteriol. 1988, 170: 1837-1842.Google Scholar
- Dukan S, Nyström T: Oxidative stress defense and deterioration of growth-arrested Escherichia coli cells. J Biol Chem. 1999, 274: 26027-26032. 10.1074/jbc.274.37.26027.View ArticleGoogle Scholar
- Le TH, Hoffmann F: Optimized production of active alpha-glucosidase by recombinant Escherichia coli. evaluation of processes using in vivo reactivation from inclusion bodies. Biotechnol Prog. 2005, 21: 1053-1061. 10.1021/bp050045+.View ArticleGoogle Scholar
- Viitanen MI, Vasala A, Neubauer P, Alatossava T: Cheese whey-induced high-cell-density production of recombinant proteins in Escherichia coli. Microb Cell Fact. 2003, 2: 2-10.1186/1475-2859-2-2.View ArticleGoogle Scholar
- Costa Gomez MF, Deschamps J, Menz DH: Solubility of dioxygen in seven fluorinated liquids. J Fluorine Chem. 2004, 125: 1325-1329. 10.1016/j.jfluchem.2004.03.013.View ArticleGoogle Scholar
- Besir H: Coomassie Staining without Alcohol and Acetic Acid. Lab Times. 2008, 6: 53-Google Scholar
- Amaral PF, Freire MG, Rocha-Leao MH, Marrucho IM, Coutinho JA, Coelho MA: Optimization of oxygen mass transfer in a multiphase bioreactor with perfluorodecalin as a second liquid phase. Biotechnol Bioeng. 2008, 99: 588-598. 10.1002/bit.21640.View ArticleGoogle Scholar
This article is published under license to BioMed Central Ltd. This is an Open Access article distributed under the terms of the Creative Commons Attribution License (http://creativecommons.org/licenses/by/2.0), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.