Production and purification of VP2 protein of porcine parvovirus expressed in an insect-baculovirus cell system
© Zhou et al; licensee BioMed Central Ltd. 2010
Received: 24 June 2010
Accepted: 10 December 2010
Published: 10 December 2010
The porcine parvovirus (PPV) VP2 protein was expressed in an insect-baculovirus cell system and was purified using Ni-NTA affinity column chromatography. The recombinant 6-His-tagged VP2 protein with molecular mass (Mr) of about 64 kDa was detected by anti-his antibody and anti-PPV serum. Electron microscopy showed that the purified VP2 protein assembled into spherical particles with diameters ranging from 20 to 22 nm. The expressed VP2 was antigenically similar to the native capsid protein according to HA and a Western blotting assay performed with polyclonal antibodies collected from an outbreak of PPV in one farm. This study provides a foundation for the application of VP2 protein in the clinical diagnosis of PPV or in the vaccination against PPV in the future.
Porcine parvovirus (PPV) causes reproductive failure in pregnant sows. The infection occurs without clinical symptoms in adults; however, the virus can cross the placental barrier during the infection and cause the death of the fetuses, stillbirths and return to estrus . More recently, PPV has gained importance as an agent able to increase the effects of porcine circovirus type 2 infection in the clinical course of postweaning multisystemic wasting syndrome (PMWS) [2, 3], which is a significant disease in global swine production . Widespread vaccination has been proposed as a cost-effective method to reduce the economical losses due to the endemic and worldwide prevalence of this virus [5, 6].
PPV is a small, non-enveloped, single-stranded, negative-sense DNA virus. Capsids of PPV are assembled from three viral proteins (VP1, VP2, and VP3). The major structural protein, VP2 is the main target for neutralizing antibodies in PPV [7, 8]. When VP2 was expressed in large amounts using the baculovirus expression vector system, it assembled into virus-like particles (VLPs) similar in size and morphology to the original virions . PPV VP2 VLPs induced antibodies against PPV in immunised pigs  and rabbits . PPV-cell or tissue-tropism determinants, host-range determinants, and determinants that confer hemagglutination properties have all been shown to be located in the capsid proteins [10–12]. It is noted that PPV VP2 was expressed by Lu et al. (2002) in pFastBac I and by Si et al. (2006) in pFastBacDUAL using insect cell-baculovirus systems and both groups demonstrated a 64 kDa band by Western-blot analysis.
Because VP2 is the main structural protein of PPV and constitutes most of the viral capsid, VP2 produced in vitro can self assemble into virus-like particles . PPV VP2 VLPs exhibited positive immunoreactivity for PPV in a commercial ELISA . Rueda et al. (2000) showed that contaminant baculovirus could be inactivated in preparations of PPV VP2 VLPs while retaining physical and immunological properties. VP2 VLPs have been produced and purified using a specific affinity Immobilized Metal Affinity Chromatography (IMAC) system for other parvoviruses such as B19  and for infectious bursal disease virus . To facilitate the use of PPV VP2 for diagnosis and vaccination, the current study attempted to identify an improved procedure for producing VP2 in vitro and for purifying this fusion protein.
There are many advantages to the use of VLPs in vaccines and for diagnosis. Compared to inactivated virus, which is currently used in vaccines, VLPs do not require the propagation of infectious virus, there is no risk of virus transmission or infection, production levels are much higher, production is cost effective, and VLPs are generally stable. The authors have previously expressed PPV VP2 in E. coli using the plasmid pET-32a (+) . VP2 expressed in bacteria had similar antigenicity to native PPV VP2, as determined by Western blot analysis using polyclonal antibodies from pigs vaccinated against PPV . PPV VP2 expressed in bacteria appears to have good immunogenicity, this is better for using as vaccine than the use as diagnosis antigen, for the antibody for E. coli in sera effects the ELISA assay. This provide us a compelling reason for expressing PPV VP2 in a baculovirus system, although baculovirus expression systems are likely to be more costly than bacterial expression systems for producing viral proteins and may present difficulty in purifying expressed proteins from insect cell and baculovirus constituents. PPV VP2 has been expressed in insect cell-baculovirus systems by a number of other groups previously [7, 9, 14, 15]. PPV VP2 expressed by baculovirus in sf9 cells produced VLPs [7, 9, 14, 15]. PPV VP2 VLPs induced antibodies against PPV in immunised pigs and rabbits . PPV VP2 VLPs exhibited positive immunoreactivity for PPV in a commercial ELISA . Rueda et al.  showed that contaminant baculovirus could be inactivated in preparations of PPV VP2 VLPs while retaining physical and immunological properties. It is noted that PPV VP2 was expressed by  in pFastBac I and by Si et al.  in pFastBacDUAL using insect cell-baculovirus systems and both groups demonstrated a 64 kDa band by Western-blot analysis. VLPs produced in baculovirus-infected insect cells could then be used as a vaccine or as a diagnostic agent to detect the antibody produced by PPV infection or vaccination . Baculovirus-infected insect cells have been used to produce VP2 VLPs of infectious bursal disease virus , and parvoviruses including PPV  and B19 . To further facilitate the use of PPV VP2 for diagnosis and vaccination, the goal of the current study was to find an improved procedure for expressing PPV VP2 in vitro and to purify the fusion protein.
2. Materials and methods
2.1. Cells, virus, and reagents
Strain 20-06 of PPV was isolated from a dead fetus delivered from a sow diagnosed with reproductive failure. HRP-labeled anti-pig serum was purchased from Sigma (St. Louis, Missouri, USA). Ni-NTA His Bind resin was obtained from Invitrogen (Carlsbad, California, USA). Prestained protein ladder was purchased from Fermentas International Inc. (Burlington, Canada). Swine anti-PPV serum samples, with serum neutralization titer, were obtained from the Harbin Veterinary Research Institute, CAAS. The serum samples were collected from an outbreak of PPV in 2008 in one farm in Heilongjiang Province.
2.2. Construction of recombinant plasmids and recombinant bacmid
Genomic DNA was extracted from the cell-cultured strain 20-06 of PPV by the classical phenol-chloroform extraction method and was used as a template to amplify the VP2 fragment by PCR. The PPV VP2 gene was amplified with the primers PPV-VP2 FD (TATGGATCCGATGAGTCATCATCACCATCACCATAGTGAAAATGTGGAACAAC) and PPV-VP2 RV (GCGTCGACTATGAGTTAGAGTTTGTATTAG). The underlined nucleotides represent BamHI and SalI restriction sites, respectively. The PCR products were digested with BamHI and SalI and subsequently cloned into the corresponding restriction sites of the pFastbac1 vector to produce the recombinant plasmid, pFastPVP2. The insert of the recombinant plasmid was confirmed by DNA sequencing.
After the recombinant pFastPVP2 donor plasmid was determined to be correct, the DNA was transformed into DH10Bac™ for transposition into the bacmid. The transposition assay and subsequent transfection steps were the same for all vectors. White colonies contained the recombinant bacmid, and therefore were selected for isolation of recombinant bacmid DNA. Before DNA was isolated, candidate colonies were streaked to ensure they were truly white. Bacmid DNA (B-pFastPVP2) was extracted by the phenol-chloroform extraction method. The recombinant Bacmid (B-pFastPVP2) was then analyzed by PCR.
2.3. Expression of the VP2 protein in sf9 cells
The recombinant baculoviruses, containing the coding sequences of VP2 with the polyhistidine tag at the N-terminus, were generated by using the Bac-to-BacTM system (Invitrogen; Luckow et al., 1993). Propagation of the recombinant virus was performed according to standard procedures (Summers et al., 2006). For production of the recombinant VP2 proteins, sf9 (Spodoptera frugiperda) cells were grown in 2-l Erlenmeyer flasks on orbital shakers (120 rpm) to a concentration of about 2 × 106 cells per ml of culture medium (30 ml growing volume) and infected with the recombinant viruses at a multiplicity of infection (MOI) of 2-3. At 72 h postinfection (p.i.), cells were collected and processed as described below. The infected cells were collected by low-speed centrifugation at 3500 × g (Hermle Labortechnik, Wehingen, Germany; swing-out rotor 4 × 750 ml) for 15 min at 4°C and solubilized in 30 ml of ice-cold lysis buffer [20 mM Tris, 0.3 M NaCl, 1.0% (v/v) Triton X-100, pH 7.4] for 15 min with gentle mixing (about 20 × 106 cells/ml). The crude cell lysate was clarified by high-speed centrifugation at 23,400 × g (Sorvall, Thermo Fisher Scientific, Waltham, MA; GSA rotor) for 20 min at 4°C. The supernatant fraction was collected, and the soluble recombinant protein products purified by IMAC as described below.
2.4. Purification of PPV VP2 protein
Cells were harvested at different times after infection, centrifuged at 200 × g for 15 min, and resuspended in 25 mM Na2HCO3, pH 8.3, at a density of 2 × 107 cells/ml; lysis was allowed to occur for 20 min. Afterward, cell debris was removed by centrifugation at 10,000 g for 15 min. The recombinant fusion protein VP2 was purified by IMAC. The clarified lysate was incubated with 3 ml of pre-equilibrated Ni2+- Streamline Chelating GelTM (Amersham Biosciences, Piscataway, NJ) on a rotating wheel for 16 h at 4°C, and was then placed in a 10-ml chromatography column (PolyPrep 0.8 by 4 cm; BioRad, Hercules, CA). Weakly bound and contaminating proteins were washed from the chelating gel by using 10× the column volume (20 mM Tris, 0.3 M NaCl, 20 mM imidazole, pH 7.4). The recombinant polyhistidine-tagged protein products were finally eluted from the packed bed with 3-4× the column volume (20 mM Tris, 0.3 MNaCl, 500 mM Mimidazole, pH 7.4). One-ml fractions were collected, and the protein contents were analyzed using a NanoDrop ND-1000 spectrophotometer (NanoDrop Technologies, Wilmington, DE).
2.5. SDS-PAGE and Western blotting
The purity and the apparent molecular weight of the recombinant VP2 specific proteins were assessed by sodium dodecyl sulfate polyacrylamide gel electrophoresis (SDS-PAGE) and immunoblot analysis. The purified proteins were separated by SDS-PAGE and were either stained with Commassie Brilliant Blue or were transferred onto nitrocellulose membranes using a wet transfer cell for Western blotting. The protein expressed 0 to 5 days after insect cells were challenged was obtained for Western blotting. The membranes were blocked with 5% skimmed milk in TBS-T (50 mM Tris-HCl, 150 mM NaCl; 0.05% Tween 20, pH 7.5) for 1 h at room temperature (RT). Swine anti-PPV sera (1:1000 dilution) or anti-His monoclonal antibody (1:5000 dilution) was added to the membranes and shaken overnight at 4°C.
The membranes were then washed three times (5 min each time) with TBS-T. Secondary antibody, either anti-swine or anti-mouse at 1:5000 dilution, was then added and incubated for 1 h. After the membranes were washed, 3,3'-diaminobenzidine (DAB) was added for colour development.
2.6. Hemagglutination assay
Following the method of Senda et al. , two-fold dilutions of samples of VP2 protein were prepared, mixed with guinea pig red blood cells, and added to the wells of a 96-well plate. After 60 minutes at 37°C, the wells were photographed.
3.1 Construction of recombinant plasmids pFastpVP2 and recombinant bacmid
3.2 Expression and purification of polyhistidine-tagged VP2 of PPV
We have previously shown that formation of chimeric VLPs of PPV fusion constructs is feasible in pET-PPV with E. coli cells (Qi T et al., 2009). The recombinant baculoviruses encoding the structural proteins VP2 of PPV N-terminally fused to a polyhistidine tag (6 × his) were engineered to simplify the overall purification process of these the viral antigens. The recombinant baculoviruses were used for infection of Sf9 insect cells according to established procedures, and the infected insect cells were collected and solubilized by treatment with a non-ionic detergent. The cell lysates were clarified by centrifugation, and the viral proteins were finally extracted from the cytoplasmic extracts by IMAC (Ni2+). After isolation, the recombinant VP2 specific fusion proteins were analyzed by SDS-PAGE, Western-blotting, and hemagglutination assay (HA).
3.3 SDS-PAGE and Western blotting
To confirm the identity of VP2 minus the his-tag tail, the purified VP2 without a His-Tag was subjected to Western blotting assay using PPV-positive pig sera. The polyclonal antibodies recognized VP2 without a His-Tag, and the band had a molecular weight of 64 KDa. The assay therefore provided evidence that the protein could be used as an efficient immunological reagent. This conclusion was supported by the HA (see next two sections).
Currently, vaccines against PPV are produced by chemically inactivating isolated virus particles grown in primary cell cultures of porcine origin. The method is both labor intensive and costly, with the additional hazard of requiring the handling of large quantities of infectious virus . Economic and safety considerations, as well as practical limitations associated with low yields of PPV particles from in vitro cultures, led us to the investigate recombinant sub-unit vaccines for PPV. The VP2 protein of PPV had been previously shown to self-assemble into virus-like particles when expressed in insect cells by baculovirus infection . In addition, the virus-like particles of PPV were found to be highly immunogenic, and breeding sows were protected against reproductive failure in PPV challenge experiments . Nonetheless, baculovirus-based systems for the production of recombinant proteins are still technically demanding, requiring sterile bioreactors that may be prohibitively costly for the production of vaccines for farm animals. Given that PPV causes serious economic losses for swine producers, development of safe, effective, and inexpensive methods for producing vaccines and diagnosing the disease is warranted.
This paper describes a method for producing the VP2 protein of PPV in an insect-baculovirus cell system. After expression was optimized, a his-tagged VP2 was obtained. The paper also describes an alternative method (IMAC) for efficient recovery of PPV VP2 and for purifying the protein using a Ni-NTA affinity column chromatography. This purification method avoids time-consuming ultracentrifugation steps such as sucrose gradient or cesium chloride gradient centrifugation. When larger amounts of recombinant proteins are needed, the purification process could be easily scaled-up by using an expanded-bed adsorption column technique. The virus-like particles formed by the fusion protein had high HA titer, could be useful as antigens for detecting PPV and could be useful for the development of a vaccine against PPV that is effective but less expensive than current vaccines .
The authors have previously expressed PPV VP2 in E. coli using the plasmid pET-32a (+) . VP2 expressed in bacteria had similar antigenicity to native PPV VP2, as determined by Western blot analysis using polyclonal antibodies from pigs vaccinated against PPV . Although PPV VP2 expressed in bacteria appears to have good immunogenicity, it is better for using as vaccine than the use as diagnosis antigen, for the antibody for E. coli in sera bothers the ELISA assay. This provide us a compelling reason for expressing PPV VP2 in a baculovirus system. The authors note a number of other studies where recombinant PPV VP2 expressed in baculovirus has been engineered with other viral antigens or immunogenic epitopes to produce multivalent vaccine candidates. The current diagnostic tests and vaccines for PPV are well established and considered to be adequate for most practical purposes; therefore the authors would like to demonstrate that any new diagnostic technology using recombinant PPV VP2 has advantages over current diagnostic tests and that any new vaccines against PPV using VP2 are superior to current vaccines in the future.
The study was supported in part by funding from the National High-tech R&D Program (863 Program-2007AA100606).
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