- Research article
- Open Access
Recombinant expression of Chlamydia trachomatis major outer membrane protein in E. Coli outer membrane as a substrate for vaccine research
BMC Microbiology volume 16, Article number: 165 (2016)
Chlamydia trachomatis is a human pathogen which causes a number of pathologies, including genital tract infections in women that can result in tubal infertility. Prevention of infection and disease control might be achieved through vaccination; however, a safe, efficacious and cost-effective vaccine against C. trachomatis infection remains an unmet medical need. C. trachomatis major outer membrane protein (MOMP), a β-barrel integral outer membrane protein, is the most abundant antigen in the outer membrane of the bacterium and has been evaluated as a subunit vaccine candidate. Recombinant MOMP (rMOMP) expressed in E. coli cytoplasm forms inclusion bodies and rMOMP extracted from inclusion bodies results in a reduced level of protection compared to the native MOMP in a mouse challenge model.
We sought to target the recombinant expression of MOMP to the E. coli outer membrane (OM). Successful surface expression was achieved with codon harmonization, utilization of low copy number vectors and promoters with moderate strength, suitable leader sequences and optimization of cell culture conditions. rMOMP was extracted from E. coli outer membrane, purified, and characterized biophysically. The OM expressed and purified rMOMP is immunogenic in mice and elicits antibodies that react to the native antigen, Chlamydia elementary body (EB).
C. trachomatis MOMP was functionally expressed on the surface of E. coli outer membrane. The OM expressed and purified rMOMP elicits antibodies that react to the native antigen, Chlamydia EB, in a mouse immunogenicity model. Surface expression of MOMP could provide useful reagents for vaccine research, and the methodology could serve as a platform to produce other outer membrane proteins recombinantly.
Chlamydia trachomatis is an obligate intracellular Gram-negative bacterium responsible for a number of pathologies. Different strains of C. trachomatis are separated into multiple serovars based on serological differences in the Chlamydia major outer membrane protein (MOMP) [1, 2]. C. trachomatis serovars A, B, Ba, and C are responsible for ocular trachoma which can cause conjunctivitis, conjunctival scarring and corneal scarring. Serovars L1, L2 and L3 are responsible for lymphogranuloma venereum, which can cause submucosa and lymph-node invasion, with necrotizing granulomas and fibrosis. Serovars D, Da, E, F, G, H, I, Ia, J, Ja and K are responsible for oculogenital disease which can cause cervicitis, urethritis, endometritis, pelvic inflammatory disease, tubal infertility, ectopic pregnancy, neonatal conjunctivitis and infant pneumonia [3, 4]. C. trachomatis infection is one of the most common sexually transmitted diseases in the world and imposes a significant medical and economic burden [5–7]. Therefore, a prophylactic vaccine is desirable to prevent C. trachomatis related diseases.
Past vaccine candidates comprised of formalin-inactivated Chlamydia trachomatis were only able to elicit short lived protection . The subunit vaccine approach has been investigated as an alternative. The Chlamydia bacterium exists outside the host cell as a metabolically inactive infectious elementary body (EB) and the Chlamydia MOMP accounts for about 60 % of the mass of the outer membrane of EBs [9, 10]. Antibodies against MOMP can neutralize infectivity of EBs and T cell epitopes have also been identified in MOMP [11, 12]. Therefore, MOMP has been an attractive subunit vaccine candidate against Chlamydia infection for many researchers [13–18]. Native MOMP (nMOMP) antigen isolated from EBs induced a protective immune response to a C. trachomatis genital challenge infection in a mouse model [14, 15]. However, development of a robust, cost-effective commercial manufacturing process based on the use of native MOMP can be challenging. Recombinant expression of a vaccine antigen is an alternative method to purification of native antigen from infected cells, and may be easier to scale-up to a commercial manufacturing level.
Chlamydia MOMPs are part of a larger family of genetically related outer membrane proteins (the OmpA family) that are heat-modifiable, surface exposed porin proteins . OmpA proteins have a structurally similar N-terminal domain that is embedded in the bacterial outer membrane. OmpA proteins have been targeted as vaccine candidates because of their surface exposure, high immunogenicity, and role in the interaction between the bacteria and their host cells. Unlike most outer membrane β-barrel proteins, MOMP is cysteine rich and was predicted to be a 16 stranded β-barrel outer membrane protein [20, 21]. Recombinantly expressed MOMP (rMOMP) has been explored as a vaccine candidate. rMOMP expressed without a leader sequence forms inclusion bodies in the cytoplasm of E. coli and rMOMP extracted from inclusion bodies resulted in a reduced level of protection compared to the native MOMP in a mouse challenge model [22, 23]. This may be due to the extracted and refolded rMOMP not having the correct conformation. Thus as an alternative, an outer membrane (OM) expressed rMOMP may attain the correct conformation and enhance the vaccine efficacy. Previous OM expression of rMOMP in E. coli resulted in significant reduction in cell viability [22, 24]. Findley et al. has shown improved surface expression of rMOMP, however did not report immunogenicity of the expressed OM rMOMP in an animal model . In this study, expression of rMOMP in E. coli outer membrane was optimized by using a number of strategies including rMOMP gene codon harmonization, utilization of low copy number vectors and promoters with moderate strength, evaluation of leader sequences and optimization of cell culture conditions. rMOMP was extracted, purified and biophysically characterized. We show here that E. coli OM expressed rMOMP possessed β-barrel structure and elicits serum antibodies that react to the native antigen, Chlamydia elementary body, in a mouse immunogenicity model.
Codon harmonization of the Chlamydia MOMP gene for recombinant expression
Nucleotide sequences of the gene encoding MOMP were retrieved from Merck internal website CMR (Comprehensive Microbial Resources) for the following strains: C. muridarum Nigg (strain MoPn) ORF TC0052 (GenBank Gene ID: 1245581; Protein link P75024.1); C. trachomatis strain D/UW-3/CX CT ORF TC_681 Serovar D (GenBank Gene ID: 884473; Protein link NP_220200.1); and C. trachomatis strain E/12–94 ORF O175_03780 Serovar E (GenBank Gene ID: 16635280; Protein link P17451). Amino acid sequences consisting of a secretion leader and the mature MOMP protein (Table 1) were codon harmonized [26, 27]. In brief, the codon usage data for Chlamydia (native host) and E. coli (expression host) were obtained from the Codon Usage Database ( http://www.kazusa.or.jp/codon/ ). For each species, the strain with the most codon usage data available was selected as a representative. The codon usage frequency for both native and expression hosts was then calculated and a reference database was generated. We first identified the amino acid residues for which the rare codons were used in the native host, and the corresponding rare codon in expression host was selected for those residues. For the remaining residues, the codon in the expression host that has the closest frequency to the corresponding codon in the native host was selected, and the harmonized gene sequence for Chlamydia MOMP was then generated. NdeI and XhoI sites were avoided in the sequences for subsequent cloning.
Cloning and expression of recombinant Chlamydia MOMP
The harmonized gene sequences with flanking NdeI and XhoI restriction enzyme sites were synthesized and cloned into the pUC57 cloning vector (Genewiz). The synthesized genes were excised from pUC57 vector through NdeI and XhoI resitriction sites. The excised DNA fragments were ligated into the pAVE029 expression vector (MSD Biologics UK) using T4 DNA ligase (Promega) for 4 h at 16 °C. Ligated plasmids were transformed into competent cells DH5α (Invitrogen) and grown on LB agar plates with 10 μg/mL tetracycline. Colonies harboring the recombinant plasmid were identified by PCR and confirmed by sequencing using pAVE029 vector specific primers for 5′end of the gene (ppop40 primer ATTCTGCATTCACTGGCCGAGG) and 3′end of the gene (T7 Term standard sequencing primer GCTAGTTATTGCTCAGCGG). The sequence-confirmed positive colonies were propagated in LB medium with 10 μg/mL of tetracycline and plasmid DNA was isolated from the cell cultures with HiSpeed Maxi Kit (Qiagen).
The recombinant plasmid DNA was transformed by electroporation into an expression host strain E. coli K12 W25113 using a Bio-Rad GenePulser. Transformed cells were plated on LB Agar plates with 10 μg/mL tetracycline and grown overnight at 37 °C. Single colonies were picked and inoculated into Cinnabar media (Teknova) with 10 μg/mL of tetracycline and grown at 37 °C with shaking at 250 rpm until OD600 reaches to mid log phase (~0.5). 0.4 mM IPTG was added into the cell culture for induction and the cell culture was incubated for 4 h at 30 °C with shaking. The cell cultures were then characterized by whole cell flow cytometry antibody binding, SDS-PAGE, and western blot analyses.
Whole cell flow cytometry antibody binding
50 μL of E. coli cell culture (at ~1x109 cells/mL) that recombinantly expresses Chlamydia MOMP was incubated with 50 μL of mouse sera generated in-house against Chlamydia EBs at a dilution of 1:250 for 1 h at room temperature in a 96 well plate. After incubation, the cells were washed with 1 mL phosphate buffered saline (PBS) and stained with 100 μL of a fluorescence labeled secondary antibody (Alexa Fluor-488 F(ab)’2 fragment of goat anti-mouse IgG (H + L), Life Technologies) at a dilution of 1:100. The stained cells were washed twice and re-suspended in PBS for flow cytometric analysis (Guava Technologies). Data analyses were performed with CytoSoft 5.3 software (Guava Technologies).
SDS-PAGE and western blot
E. coli cell culture (~1x109 cells) that recombinantly expresses Chlamydia MOMP was treated with SDS loading buffer with reducing agent (Invitrogen). Samples were applied to NuPAGE (Invitrogen) gel electrophoresis. NuPAGE gel was stained with Gel Code Blue staining solution (Pierce). For western blot, samples were applied to gel electrophoresis and then electro-transferred onto nitrocellulose membranes (Life Technologies). The membranes were incubated with mouse sera against Chlamydia EBs (or other specific primary antibodies) followed by a fluorescence conjugated goat anti-mouse secondary antibody (IRDye 680LT, Licor). Image was acquired and analyzed by a LI-COR Odyssey imaging system.
Purification of Chlamydia MOMP
E. coli cell culture was grown in Cinnabar media (Teknova) and induced by IPTG as described above. Cell culture was harvested by centrifugation at 12,000 x g for 15 min. Cell pellets were weighed and resuspended in 9 volumes (v/w) of 50 mM Tris-Cl pH 8.0 buffer with EDTA free protease inhibitor (Roche, 1 tab per 100 mL buffer). Cells were disrupted by microfluidization and undisrupted cells were pelleted and removed by centrifugation at 9700 x g for 15 min. Membrane fraction was pelleted by centrifugation of the cleared disrupted cells at 23800 x g for 90 min and washed with high salt buffer (1 M NaCl, 0.05 % tween20) followed by another centrifugation at 23800 x g for 90 min. To remove the bacterial inner membrane, washed membrane fraction was resuspended in buffer A (20 mM Tris-Cl pH 8.0, 1 mM EDTA) with 1 % Triton X-100, incubated at room temperature for 15 min followed by ultracentrifugation at 120,000 x g for 40 min. To remove bacterial outer membrane proteins other than recombinant MOMP, pellets were resuspended by buffer A with 3 % β-octyl-glucoside, incubated at room temperature for 1 h followed by ultracentrifugation at 120,000 x g for 40 min. rMOMP was extracted by resuspending the pellets in buffer A with 1 % sarkosyl and 5 mM DTT, incubated at room temperature for 2 h followed by ultracentrifugation at 120,000 x g for 40 min. Extracted rMOMP was subjected to size exclusion chromatography (Sephacryl S300, GE healthcare) in a buffer containing 10 mM Hepes pH 7.3, 150 mM NaCl, 0.1 % zwittergent 3–14. Eluted rMOMP was further purified with ion exchange chromatography (Hitrap Q FF, GE healthcare). Purified rMOMP fractions were pooled and stored at 4 °C. Native MOMP was purified from infected HELA cells similarly as previously described . Briefly, nMOMP was extracted from intact Chlamydia-infected HELA cells using CHAPS and zwittergent 3–14 with 100 mM DTT and sonication, and further purified with hydroxyapatite chromatography, tangential flow filtration, and anion exchange chromatography.
Circular dichroism spectroscopy
Circular dichroism spectra were acquired on a Chirascan spectrometer (Applied Photophysics LtD, UK). Samples were analyzed undiluted using a quartz cuvette with 0.5 mm pathlength. The temperature control was set to 20 °C. The bandwidth was set to 1 nm and data points between 200 nm and 280 nm were acquired in 1 nm intervals. Scans below 200 nm exceeded the allowable photomultiplier voltage and were not recorded. Sample and buffer spectra were acquired after 10 min of temperature equilibration applying three technical replicates, respectively. Average buffer spectra were subtracted from sample spectra. Resulting data points were smoothed with the Savitzky-Golay algorithm (polynomial order 2, two data points to left and right) using the Origin Pro 7.5 SR7 software package (Origin Lab Corporation).
Cell culture and propagation of Chlamydiae
All cell lines and Chlamydia strains were obtained from ATCC (Manassas, VA). HeLa 229 cells were used for propagation of all strains. HeLa 229 cells were grown in Eagle’s Minimal Essential Medium (ATCC) supplemented with 10 % heat-inactivated fetal bovine serum (Hyclone), 50 μg/mL vancomycin (Sigma), and 10 μg/mL gentamicin (Gibco). Host cells were seeded into tissue culture flasks at a cell density of 5 × 105 cells/mL and incubated overnight at 37 °C in 5 % CO2 to achieve a confluent monolayer. Cell monolayers were infected with C. trachomatis (Ct) strain D/UW-2/Cx stock diluted in sucrose–phosphate–glutamate (SPG) buffer and cultured for 72 h. The Chlamydiae were harvested from the infected cells and purified by centrifugation through 30 % Renograffin (Bracco Diagnostics) and stored frozen at -80 °C.
Mouse immunization and challenge
Female C57BL/6 mice (Taconic Farms) were used at 6 to 8 weeks of age, and food and water were provided ad libitum. All animal procedures were in accordance with government and institutional guidelines for animal health and well-being, and were approved by the Merck Institutional Animal Care and Use Committee.
Animals were immunized by subcutaneous (s.c.) routes with rMOMP or nMOMP (10 μg/mouse/immunization) in combination with an adjuvant containing 50 μg CpG and 70 % (w/v) Montanide ISA 720 VG (SEPPIC Inc., Coley Pharmaceutical Group). Live EB groups were immunized with 1x106 EB in SPG per mouse by intraperitoneal (i.p.) route. Adjuvant control groups were administered with a combination of CpG and Montanide ISA 720 VG only. Immunizations were administered on days 0, 20 and 30.
Prior to the first immunization and two weeks following the final immunization, tail bleeds were performed with blood collected in BD Microtainer® Serum Separator Tubes (Becton, Dickinson and Company). Blood samples were centrifuged at 6,000 rpm for 5 min and serum was transferred to a microcentrifuge tube.
At approximately 2 weeks following the last immunization, progesterone (medroxyprogesterone acetate, Depo-Provera; Pfizer) was administered subcutaneously (2.5 mg/dose) at 10 and 3 days before challenge. Mice were challenged intravaginally (approximately 1 month following the last immunization) by direct instillation of 10 μL of SPG containing 1x105 Ct serovar D EBs. The vaginal vault and ectocervix were swabbed using a microfiber swab (Fisher) on days 7, 11, 14, 18, and 21 (or a combination of these time points) following challenge.
Swabs were placed into a 1.5-mL tube containing 2 sterile glass beads (5 mm diameter) and 300 μL of Chlamydia isolation medium (Trinity Biotech) on ice. Bacteria were eluted from the swabs and separated from cells by vortexing for 60 s. 100 μL of eluted cells/bacteria were plated onto a processing cartridge containing 100 μL of PBS and stored at -70 °C until DNA extraction.
Primer, probe and real-time PCR
DNA from genital swab samples was extracted using the MagNA Pure 96 DNA and Viral NA small volume kit (Roche) on the MagNA pure machine (Roche) according to the manufacturer’s instructions.
The oligonucleotide primer set was designed for detection of all species of Chlamydiae. The sense primer, 16S DIR 5′-CGCCTGAGGAGTACACTCGC-3′, and anti-sense primer, 16S Rev 5′-CCAACACCTCACGGCACGAG-3′, were designed to amplify a 208-bp fragment of the Chlamydial 16S ribosomal subunit gene, conserved across Chlamydia strains and serovars. Primers were obtained from Sigma Genosys (The Woodlands, TX), and the probe, 16S Fam-5′-CACAAGCAGTGGAGCATGTGGTTTAA-3′ Tamra, was synthesized by Applied Biosystems, (Foster City, CA).
The 50-μL reaction mixtures consisted of 1× QuantiTect Multiplex PCR master mix without ROX (Qiagen), 100 nmol/L 16S probe, 200 nmol/L primer 16S DIR, 400 nmol/L primer 16S Rev, 30 nmol/L ROX reference dye, and 5 μL of sample DNA. Nontemplate controls consisting of the reaction master mix, primers, and probe, but no DNA, were included in each assay run. Reaction conditions were set as follows: 1 cycle at 95 °C for 15 min, followed by 40 cycles at 94 °C for 1 min and at 60 °C for 1 min. Thermal cycling, fluorescent data collection, and data analysis were performed using the Stratagene Mx3005P system (Stratagene) according to the manufacturer’s instructions.
Detection of serum antibody and isotype levels by ELISA
Serum was analyzed by an enzyme-linked immunosorbent assay (ELISA). Nunc ™ C96 Maxisorp Immunoplates (Thermo Scientific) were coated with 50 μL of 1 μg/mL C. trachomatis Serovar D EBs in PBS and refrigerated overnight. The plates were washed three times with 0.05 % Tween-20 (Fisher Scientific) in PBS (PBS-T). The wells were blocked with 5 % HyClone® fetal bovine serum (Thermo Scientific) in PBS at 200 μL/well for 1 h at room temperature and washed three times with PBS-T. Serum was diluted in 5 % FBS in PBS at a 1:500 dilution. Serially diluted sera were added to the plate, incubated for 2 h at room temperature and the plates were washed three times with PBS-T. HRP-conjugated secondary antibodies (Goat anti-mouse IgG, Fcγ fragment specific; Goat Anti-mouse IgG, Fcγ Subclass 1 specific; or Goat Anti-mouse IgG, Fcγ Subclass 2c specific; Jackson ImmunoResearch Laboratories) were diluted in 5 % FBS in PBS at 1:6,000, 1:6,000, or 1:2,000 dilution, respectively. The diluted secondary antibodies were added at 100 μL/well, incubated for 1 h at room temperature and the plates were washed three times with PBS-T followed by three times with PBS. Room temperature BD Opt EIA™ TMB Substrate Reagent Set (BD Biosciences) was mixed and filtered through a 0.22um CA filter unit (Corning), and 100 μL was added to each well and incubated for 10 min at room temperature. The reaction was stopped with 100 μL/well of 2 M H2SO4 (Fisher Scientific). The optical density (OD) was read at 450 nm on a SpectraMax® M5 (Molecular Devices). The cutoff OD for each post-immunization serum was calculated as two times of the OD450 of the corresponding pre-immunization serum. ELISA titers were determined by linearly interpolating between the sequential log dilutions that bracket the cutoff OD, where the dependent variable is the OD response and the independent variable is the log dilution. The resulting dilution is then back transformed to obtain the reported titer. The reported titer is the estimated dilution of serum that results in a response equivalent to the cutoff OD.
Expression of recombinant Chlamydia MOMP
To improve recombinant protein expression in a heterologous host, Angov et al. developed an algorithm termed “codon harmonization” that best approximates codon usage frequencies from the native host and adjusts these for use in the heterologous system [26, 27]. We performed either codon harmonization or standard codon optimization on a recombinant Chlamydia muridarum (Cm) MOMP gene and evaluated outer membrane expression with a whole cell flow cytometry antibody binding assay using in-house generated polyclonal mouse sera against Chlamydia EB. Both codon type genes were expressed in a pET vector expression system and with a MOMP native leader sequence. We observed that codon harmonization resulted in ~2 fold increase in geomean fluorescence intensity (GFI) compared to the standard host codon optimized gene (Fig. 1). Therefore, codon harmonized genes were used in subsequent expression evaluations (data below) to further improve rMOMP OM expression.
Expression vector optimization
A panel of E. coli expression vectors were evaluated to further increase the surface expression level of rMOMP (Table 2). Recombinant C. trachomatis Serovar E (CtE) MOMP with a PelB leader sequence was used in this evaluation. The key elements that could affect the OM expression include promoter strength and vector copy number. We compared vectors with high, medium or low copy numbers, and promoters of high, moderate or titratable strength. We found that either a strong promoter or a high vector copy number limited the surface expression of rMOMP using whole cell flow cytometry antibody binding assay (Table 2). High rMOMP surface expression can only be achieved with a combination of moderate promoter and a low vector copy number (such as pAVE029), suggesting that lower transcription level is preferred. Consistent, rMOMP OM expression can be obtained with a pACYDuet vector when we used a host strain with a controllable RNA polymerase level to reduce the rMOMP mRNA transcription rate.
Secretion leader sequence optimization
There are several advantages of secretory production of recombinant membrane proteins compared to cytosolic production. The N-terminal amino acid residue of the secreted product can be identical to the natural gene product after cleavage of the signal sequence by a specific signal peptidase. Also, there appears to be much less protease activity in the periplasmic space than in the cytoplasm . In addition, disulfide bonds formation can be facilitated because the periplasmic space provides a more oxidative environment than the cytoplasm . Enhanced OM insertion and prevention of periplasmic space inclusion bodies were investigated. Two amino acids at the C-terminus of CtD-MOMP (C. trachomatis Serovar D) were modified to improve the binding to the E. coli β-barrel assembly complex protein (BamA), which recognizes its outer membrane protein substrates by a species-specific C-terminal signature motif . However, we did not observe a difference in surface expression levels between the wild type CtD-MOMP and the C-terminus modified CtD-MOMP sequences (unpublished observations). Different secretion leader sequences reported to improve the OM localization of the target protein were investigated by using a whole cell flow cytometry antibody binding assay (Table 1). pAVE029 expression vector was used in this evaluation for Cm-MOMP, CtE-MOMP and CtD-MOMP. Among tested leader sequences, E. coli OmpA and OmpP leaders, leader sequences from the omptins (SopA, PgtE, and Pla), and PelB leader all resulted in detectable surface expression of rMOMP. Native Cm-MOMP leader was able to direct the OM expression for Cm-MOMP, however, neither of native CtD- or CtE-MOMP leaders resulted in the surface expression of rMOMP.
Expression condition optimization
Surface expression of rMOMP has been associated with toxicity to the host cell, resulting in a low yield [22, 24, 25]. We evaluated a variety of cell culture conditions with the pAVE029 expression system, including induction time and temperature, cell density at induction, and cell culture medium (Fig. 2). rCtE-MOMP with a PelB leader sequence was used in this evaluation. We performed induction for 4 h, 6 h and 16 h under four different temperatures: 16 °C, 25 °C, 30 °C and 37 °C. We found that 4 h and 6 h resulted in comparable rMOMP OM expression levels while no expression was observed following 16 h induction at any of the temperatures tested (Fig. 2a). Induction for 4 or 6 h at 37 °C or 30 °C resulted in higher surface expression of rMOMP than 25 °C and no detectable surface expression was observed at 16 °C (Fig. 2a). We also observed cell fragility at 37 °C (but not at 30 °C), which was indicated by a decrease in OD590 after induction (Fig. 2b). We performed induction at different cell densities and found that it dramatically impacts the rMOMP surface expression. The highest rMOMP expression was obtained with an induction OD590 of ~0.5, while expression dropped with an induction OD590 of ~0.8, while little or no surface expression of rMOMP was observed with an induction OD590 of 1.2 or higher (Fig. 2c). We evaluated seven cell culture mediums and interestingly, the culture medium used had a large impact on rMOMP OM expression (Fig. 2d). Low levels of rMOMP OM expression were observed with LB medium, 0.2 % lactose auto induction medium, 2YT medium with 1 % glucose, and the chemically defined Azura medium. The highest rMOMP OM expression (GFI ~300 to 400 in the whole cell flow cytometry antibody binding assay) was obtained with growth in Cinnabar medium. We obtained very high level of periplasmic rMOMP expression with Progro medium, however, no surface expression was observed. IPTG concentration for induction was also evaluated and comparable rMOMP OM expression was observed with 0.1 mM to 1 mM IPTG (unpublished observations). Therefore, all expression studies described here were induced by addition of 0.4 mM IPTG.
In summary, optimal conditions for rCtE-MOMP OM expression was found to be induction for 4 h at 30 °C in cells grown in Cinnabar medium when cell density (OD590) reaches ~0.5 (Fig. 3). Three different rMOMP proteins (Cm, CtD and CtE) have been successfully expressed on E. coli outer membrane under these conditions. rCtE-MOMP with a PelB leader sequence was used for the subsequent purification, characterization and immunogenicity studies in this manuscript.
Purification and characterization of recombinant Chlamydia MOMP
Following optimization of rCtE-MOMP OM expression, the recombinant protein was purified. Harvested E. coli cells expressing rMOMP were disrupted by microfludization and the membrane fraction containing rMOMP was pelleted by ultra-centrifugation. Washing the membrane fraction with high salt buffer further removed residual soluble cellular proteins. A subsequent wash with a buffer containing 1 % Triton X-100 detergent removed the bacterial inner membrane and a wash with a buffer containing 3 % β-octyl-glucoside detergent removed certain bacterial outer membrane proteins other than recombinant MOMP. A variety of detergents were evaluated for extraction of rMOMP from the outer membrane. We found that sarkosyl (an anionic detergent) was the most efficient, followed by foscholine-14 (a lipid like zwitterionic detergent) and zwittergent 3–12. DTT was required for extraction of rMOMP. Sarkosyl extracted rMOMP was further purified by size exclusion and ion exchange chromatography. Purified protein concentration was measured by amino acid analysis and the total yield of purified rMOMP is about ~6 mg per liter of cell culture (mean from three preparations).
The purified rCtE-MOMP migrates very similarly to the native CtE-MOMP (nCtE-MOMP) that was purified from Chlamydia EBs on a SDS-PAGE gel (Fig. 4a and b). It appears that compared to nMOMP, rMOMP has a slightly higher amount of dimeric and oligomeric forms that are SDS-resistant and independent of disulfide reductants (Fig. 4b). A western blot using antisera generated against outer membrane vesicles from the host E. coli strain without the recombinant MOMP gene showed that the purified rMOMP contained some co-purified E. coli host proteins (Fig. 4c, sample 2), and the purity is estimated to be about ~70 % as determined by mass spectrometry (unpublished observations). We have attempted to improve the purity of the preparation by using different extraction and purification methods, however, were unable to further remove the co-purified host proteins when the rMOMP protein is expressed without an affinity tag. Complete processing of the PelB leader sequence was confirmed by mass spectrometry (unpublished observations). The endotoxin level in the final purified protein sample is undetectable with an anti-E.coli lipo-oligosaccharide (LPS) antibody on western blot (Fig. 4d, sample 2).
To investigate whether the recombinantly expressed rCtE-MOMP possessed β-strand secondary structure, we performed circular dichroism (CD) analysis. CD spectra of nMOMP and rMOMP both have a peak at ~215 nm which is the signature of β-strand structure (Fig. 5). Interestingly, rMOMP appears to have a significant higher mean molar ellipticity as compared to the native MOMP. One possible explanation is that the recombinant and native MOMPs were extracted and purified differently, even though both were exchanged into the same final storage buffer. The co-purified E. coli host proteins might also contribute to the difference observed.
Mouse immunogenicity study
Our next goal was to evaluate the immunogenicity of rCtE-MOMP in mice. Female C57BL/6 mice were immunized three times by subcutaneous (s.c.) routes with purified nCtE-MOMP or rCtE-MOMP (10 μg/mouse/immunization) in combination with an adjuvant containing CpG and Montanide on days 0, 20 and 30. A positive control group was immunized with 1x106 live EB per mouse by intraperitoneal (i.p.) route. A negative control group (adjuvant control) was administered with a combination of CpG and Montanide only.
Post-immunization mouse serum was analyzed by ELISA with CtD EBs as the coating antigen (Fig. 6). The rMOMP immunized mice have comparable (no statistical difference) IgGFcγ titers to the nMOMP immunized group (Fig. 6a). We also tested subtypes of the antibodies to evaluate whether the vaccine responses are Th1 or Th2 biased. rCtE-MOMP elicited similar antibody profiles to the nMOMP immunized group (Fig. 6b). These data suggested that the OM expressed rMOMP elicits a similar antibody response in mice that react to the native Chlamydia EB antigen, as compared to the native MOMP.
Two weeks following the last immunization, mice were challenged intravaginally with CtD EBs. The vaginal vault and ectocervix were swabbed on multiple time points (day 7 to day 21) following challenge. Previously, a comparative analysis between a real-time quantitative PCR (qPCR) and inclusion forming unit (IFU) measurement was performed and no major differences between the two assays were observed in monitoring infections . IFU analyis is more labor intensive, more subjective, and not as high-throughput as qPCR. Therefore, qPCR assay was chosen for evaluating our vaccines in this study. rCtE-MOMP elicited significant reduction in Chlamydial shedding compared to the adjuvant only control group (P < 0.01) (Fig. 7). Moreover, the amount of shedding after bacterial challenge in mice immunized with rMOMP was comparable (similar bacterial load post-challenge) to the amount observed in the nMOMP immunized group (Fig. 7).
E. coli has been the most prominent host system for production of recombinant proteins [29, 32]. However, the E. coli cytoplasmic expression system does have some drawbacks. It is not suitable for production of certain proteins, for example, proteins containing complex disulfide bonds. Overexpressed proteins are often produced in the form of inclusion bodies, from which biologically active proteins can only be recovered by complicated denaturation and refolding processes that often have a low recovery. Overexpression of membrane proteins adds additional complexity. We applied a variety of techniques, including the adjustment of codon usage bias, evaluation of different promoters and vectors with different copy numbers to regulate the level of gene transcription, evaluation of different leader sequences to guide the secretion and insertion of the target protein into outer membrane, and evaluation of cell culture medium and optimization of cell culture conditions. In this paper, we demonstrated significant improvement for the recombinant expression of Chlamydia MOMP with some of the techniques mentioned above.
Codon usage is a reflection of the relative amounts of cognate aminoacyl tRNAs accessible in the cytoplasm. The synonymous codon usage in all the organisms displays a bias—some codons are used frequently, while others are rarely used. Like others cellular systems, E. coli also shows disparities for synonymous codons where in general major codons are predominantly present in highly expressed genes and rare codon occurs in low level expressed genes. This disproportion of codon frequency preferences becomes highly critical for recombinant expression systems, and can lead to mRNA instability, ribosomal stalling, translation errors or premature translational terminations, and ultimately failure to express recombinant genes by heterologous expression hosts. Reported studies indicated that folding and post-translational modifications for both membrane and soluble proteins are also susceptible to synonymous codon usage . Recent studies have shown that codon harmonization, a methodology that matches the codon usage in the recombinant host closely to the usage in the gene’s native organism including the usage of low abundance rare codons (unlike “codon optimization” methodology that often excludes rare codons), can significantly improve the yield and solubility of recombinant proteins [26, 27]. Presumably by this codon selection, pauses in the translation process are incorporated which leads to improved protein folding and efficient protein biosynthesis. In this study, we adapted the concept of codon harmonization and demonstrated successful recombinant expression of the Chlamydia MOMP, a cysteine-rich, full-length β-barrel integral membrane protein.
Outer membrane expression of β-barrel proteins in gram-negative bacteria is complicated, involving translation, secretion across inner membrane into the periplasmic space in the unfolded state, simultaneous cognate chaperone assisted folding and insertion into the outer membrane via β-barrel assembly machinery (BAM) complex [34, 35]. Here, we evaluated different promoters, vectors, leader sequences and cell culture conditions for increased outer membrane rMOMP expression. Our data suggested that the combination of a moderate promoter and a low vector copy number greatly improved rMOMP surface expression. We hypothesized that slower transcription and therefore slower translation is optimal for rMOMP OM expression as it provides ample time to allow the newly synthesized protein to be transported into the periplasmic space, properly fold there and translocate onto the outer membrane, resulting in an increased level of surface expression. We have also evaluated different secretion leader sequences, as the efficiency of protein secretion is affected by the leader sequence, even though many prokaryotic and eukaryotic leader sequences are functionally interchangeable. We found that leader sequences originated from the expression host E. coli, such as OmpA and OmpP, drove higher levels of rMOMP surface expression as compared to the native Chlamydia leader sequences. Surface expression of rMOMP has been associated with toxicity to the host cell [22, 24]. As we need to strike a balance between rMOMP OM expression and the host cell viability, many factors need to be optimized to achieve the best outcome, including optimal cell culture medium, induction of protein expression on or before mid-log phase, and induction at a certain temperature. Our data suggested that the higher surface expression level of a membrane protein such as MOMP can be achieved with a combination of molecular biology and cell culture techniques.
A well-known step along the protein folding pathway that often requires catalysis in vivo is the cis/trans isomerization of prolyl-iminopeptide bonds . Four peptidyl-prolyl cis/trans-isomerases (PPIases), SurA, PpiD, FkpA and PpiA, have been described for the isomerization role in periplasm of E. coli . We hypothesized that co-expression of these enzymes might improve the efficiency of periplasmic folding of rMOMP and therefore enhance its OM expression level. In addition, proper disulfide bond formation is also presumed to be critical for correct folding of MOMP, a cysteine-rich protein. Both DsbA and DsbC, members of the thioredoxin superfamily, are critical for catalysis of correct disulfide bonds . Another future attempt will be to test the OM expression of rMOMP in an E. coli host strain that overexpresses these oxidoreductases.
Refolded rMOMP from E. coli inclusion bodies resulted in a reduced level of protection compared to the native MOMP in a mouse challenge model, suggesting that correct conformation of MOMP is required for protective immune responses . Consistent with this finding, rMOMP extracted from inclusion bodies and refolded in vitro elicited a significant lower antibody titer against Chlamydia EB (unpublished observations). We showed here that OM expressed rMOMP maintained β-strand secondary structure as expected and elicited a comparable antibody response in mice that react to the native Chlamydia EB antigen, as compared to the native MOMP. Whether the native tertiary structure is preserved in OM expressed rMOMP remains to be determined, as no molecular structures of either native MOMP or recombinant MOMP are available to date. However, our data suggested that the OM expressed rMOMP at least contains some epitopes in their native forms.
Strains of Chlamydia trachomatis human serovars have been used as the challenge strain in murine genital tract models, even though intravaginal inoculation with human serovars typically results in a mild genital tract infection of short duration and lower bacterial burdens [39, 40]. We used C. trachomatis serovar D as the challenge strain in our mouse immunogenicity model, and demonstrated that immunization with either native or OM expressed rMOMP resulted in similar low levels of post-challenge bacterial burden, consistent with the comparable antibody responses elicited from rMOMP and nMOMP immunizations. A recent study in adaptive immune deficient mice which lack mature T and B cell immunity but maintain functional innate immune effectors showed that C. muridarum infection was unable to be resolved but C. trachomatis infection was spontaneously cleared, suggesting a possibility that innate immunity is sufficient to clear the C. trachomatis infection in mice . Therefore, the comparison of vaccine efficacy between recombinant and native MOMPs needs to be also evaluated in the more stringent C. muridarum mouse challenge model to further confirm the role of adaptive immune response. However, the techniques that we applied to successfully achieve recombinant Chlamydia MOMP outer membrane expression can serve as a platform to produce other outer membrane proteins as vaccines or drug candidates and useful reagents for research, as many of these are membrane proteins.
C. trachomatis MOMP is an immunodominant surface protein of crucial importance in the immune response to Chlamydia infection and also a major subunit vaccine target. Recombinant MOMP expressed in E. coli cytoplasm forms inclusion bodies and rMOMP extracted from inclusion bodies results in a reduced level of protection compared to the native MOMP in a mouse challenge model. Here we demonstrated successful recombinant expression of MOMP on the E. coli outer membrane achieved with a variety of techniques, including codon harmonization, utilization of low copy number vectors and promoters with moderate strength, suitable leader sequences and optimization of cell culture conditions. The E. coli OM expressed and purified rMOMP is immunogenic in mice and elicits antibodies that react to the native antigen, Chlamydia elementary body. Using C. trachomatis serovar D as the challenge strain in our mouse immunogenicity model, we demonstrated that immunization with either native or OM expressed rMOMP resulted in similar low levels of post-challenge bacterial burden. Surface expression of rMOMP on E. coli OM could provide useful reagents for vaccine research, and the methodology could also serve as a platform to produce other outer membrane proteins.
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The authors would like to thank Jing Lin, Hui Xu, Ivette Caro-Aguilar, Andy Xie and Melanie Horton for technical assistance; Kalpit Vora and Danilo Casimiro for critical review of the manuscript and Kevin Issett for helpful discussions. We also would like to thank all the scientists in MRL ID/Vaccines Discovery who have supported this work.
The research was fully funded by Merck and Co., Inc. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
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All data generated or analyzed during this study are included in this published article and its supplementary information files.
ZW, MAB, RMK, PK, ED, PQ, BJL, DDN, JCC, ST, JMS and LZ performed the experiments. ZW, MAB, RMK, PK, ED, JMS, ASE, CTP and LZ analyzed the data. ZW, CTP and LZ wrote the manuscript. All authors read and approved the final manuscript.
All co-authors work for Merck & Co., Inc., Kenilworth, NJ, as indicated on the title page of the manuscript. Lan Zhang, Zhiyun Wen, Craig T. Przysiecki, Puneet Khandelwal and Ping Qiu are currently applying for a patent relating to the content of the manuscript (International Application No. PCT/US15/060780).
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All animal procedures were in accordance with government and institutional guidelines for animal health and well-being, and were approved by the Merck Institutional Animal Care and Use Committee.
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Wen, Z., Boddicker, M.A., Kaufhold, R.M. et al. Recombinant expression of Chlamydia trachomatis major outer membrane protein in E. Coli outer membrane as a substrate for vaccine research. BMC Microbiol 16, 165 (2016). https://doi.org/10.1186/s12866-016-0787-3
- Chlamydia trachomatis
- Outer membrane expression