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Acellular Pertussis vaccines against whooping cough caused by Bordetella pertussis present a much-improved safety profile compared to the original vaccine of killed whole cells. The principal antigen of acellular Pertussis vaccine, Pertussis Toxin (PT), must be chemically inactivated to obtain the corresponding toxoid (PTd). This process, however, results in extensive denaturation of the antigen. The development of acellular Pertussis vaccines containing PTd or recombinant PT (rPT) with inactivated S1, Filamentous Hemagglutinin (FHA), and Pertactin (PRN) has shown that the yield of PRN was limiting, whereas FHA was overproduced. To improve antigen yields and process economics, we have constructed strains of Bordetella pertussis that produce enhanced levels of both rPT and PRN.
Three recombinant strains of Bordetella pertussis were obtained by homologous recombination using an allelic exchange vector, pSS4245. In the first construct, the segment encoding PT subunit S1 was replaced by two mutations (R9K and E129G) that removed PT toxicity and Bp-WWC strain was obtained. In the second construct, a second copy of the whole cluster of PT structural genes containing the above mutations was inserted elsewhere into the chromosome of Bp-WWC and the Bp-WWD strain was obtained. This strain generated increased amounts of rPT (3.77 ± 0.53 μg/mL) compared to Bp-WWC (2.61 ± 0.16 μg/mL) and wild type strain (2.2 μg/mL). In the third construct, a second copy of the prn gene was inserted into the chromosome of Bp-WWD to obtain Bp-WWE. Strain Bp-WWE produced PRN at 4.18 ± 1.02 μg/mL in the cell extract which was about two-fold higher than Bp-WWC (2.48 ± 0.10 μg/mL) and Bp-WWD (2.31 ± 0.17 μg/mL). Purified PTd from Bp-WWD at 0.8-1.6 μg/well did not show any toxicity against Chinese hamster ovary (CHO) cell whereas purified PT from WT demonstrated a cell clustering endpoint at 2.6 pg/well.
We have constructed Bordetella pertussis strains expressing increased amounts of the antigens, rPT or rPT and PRN. Expression of the third antigen, FHA was unchanged (always in excess). These strains will be useful for the manufacture of affordable acellular Pertussis vaccines.
Pertussis or whooping cough is a severe respiratory disease resulting from colonisation of the upper respiratory tract by the causative organism Bordetella pertussis . Vaccines have been available for decades, comprising killed whole cells of B. pertussis that are chemically detoxified and formulated with Diphtheria and Tetanus antigens. They are administered as a trivalent Diphtheria-Tetanus-Pertussis combination, or in newer combinations with HBV and Hib, providing additional immunity against Hepatitis B and Haemophilus influenzae type b invasive disease, respectively . The use of whole-cell Pertussis vaccines has been reduced, discouraged, or even banned in a few countries, due to the whole-cell vaccine's questionable safety profile, resulting from high level of endotoxin and other bacterial toxins associated with killed whole cells [3,4].
Acellular Pertussis vaccines (so-called because they do not contain whole cells but only partially- or extensively-purified bacterial antigens), were introduced in Japan in 1981 . The higher purity of the component antigens in acellular Pertussis vaccines provided an improved clinical safety profile. These vaccines were introduced in the mid 90 s in other industrialized countries after extensive clinical trials that demonstrated their safety and efficacy . A broader introduction by the WHO into the Expanded Program of Immunization was, however, hampered by the significantly higher cost of acellular Pertussis vaccines.
A major virulence factor of B. pertussis is Pertussis Toxin (PT) [7,8] and pertussis toxoid (PTd) is still the principal antigen in acellular vaccines . Unlike Diphtheria and Tetanus toxins (that can be inactivated by simple treatment with formaldehyde), PT proved more difficult to be inactivated by chemical means . At present, different inactivation processes are in use for commercial manufacture of acellular Pertussis vaccines. Unfortunately, all of them cause extensive denaturation of PT by their chemical treatments.
Two candidate vaccines have been tested using a genetically-inactivated toxin (rPT) [10-12] and one of these candidates was included in a field efficacy trial [11,12]. This vaccine was obtained by introducing two mutations into the catalytic subunit S1 of PT, causing abolition of the enzymatic activity of S1 and thus providing complete absence of toxicity of native PT. This vaccine was formulated with 5 μg rPT, 2.5 μg FHA and 2.5 μg PRN and was compared with another vaccine manufactured using classical chemical inactivation, comprising 25 μg PTd, 25 μg FHA and 8 μg PRN. The two vaccines had identical safety and efficacy results in this trial . It was understood that the efficacy obtained with a lower dose of rPT and the other antigens was a result of using native antigens that included native FHA and PRN as the latter also required chemical treatment to inactivate residual traces of toxin when the antigens were derived from wild type B. pertussis.
Unfortunately, the vaccine described above, containing rPT, is not currently available due to unresolved intellectual property issues at the time of planned commercial introduction. Nevertheless, it is clear that the genetically-engineered approach to detoxification of Pertussis vaccine antigens is an essential element for the design of affordable acellular Pertussis vaccines, as intellectual property rights are expiring.
The vaccines referred to above contained three purified antigens derived from B. pertussis cultures: PTd or rPT, FHA and PRN. PT and even more so PRN are limiting antigens in B. pertussis cultures, while FHA is naturally overproduced. Alternative expression systems exist for increasing level of limiting B. pertussis vaccine antigens. PRN was expressed in high yield from recombinant Escherichia coli or from the recombinant yeast, Pichia pastoris [14,15]. PT subunits were expressed in E. coli, but unfortunately these failed to assemble into the mature toxin and were insufficiently immunogenic to be considered as potential vaccine candidates . It is now understood that assembly and secretion of the mature toxin requires several auxiliary genes that were discovered more recently, and these genes are part of the ptl section of the ptx-ptl operon .
In this publication, we report the construction of recombinant B. pertussis strains expressing increased levels of rPT or rPT and PRN. These strains were generated by a multiple allelic- exchange process: insertion of the mutations that abolish the catalytic activity of subunit S1, insertion of a second copy of the ptx cluster of the five PT structural genes of the ptx-ptl operon with their promoter and terminator into an abandoned gene elsewhere on the chromosome, then insertion of a second copy of the prn gene into a second inactive gene locus. The organization of ptl auxiliary genes present in the ptx-ptl operon was not modified. Enhanced production of rPT and PRN by manipulation of gene copy number has been largely used with multi-copy plasmid vectors and reported to enhance the production of bacterial toxins [18,19], in particular PT . However, genes tandemly repeated in this way may have significantly negative consequences on strain genetic stability in a GMP-regulated, vaccine-manufacturing environment. In addition, PRN expression could also be increased by manipulation of the PRN promoter .
The allelic-exchange vectors used in earlier B. pertussis recombinant strains require mutations on the chromosome, particularly the mutation affecting rpsL that results from selection of spontaneous streptomycin-resistant mutants as required in earlier allelic-exchange procedures . Such mutations affecting housekeeping genes may impair virulence, hence the expression of virulence factors including PT, FHA and PRN. In contrary, pSS4245 used in this study harbours streptomycin resistant gene from Tn5 which is functional in B. pertussis but not in E. coli, hence streptomycin was used to select against E. coli donor cell and I-SceI nuclease activity in the plasmid was then functioned as the counter selectable marker in the recombinant B. pertussis through subsequent homologous recombination and does not require or leave auxiliary mutations. The strains reported here produce unaltered levels of the other antigens in particular FHA. These constructs will prove useful for the manufacture of affordable human acellular Pertussis vaccines.
To introduce the two mutations R9K and E129G into the S1 subunit, a two-stage approach was used to avoid the possibility of recombination in the region between the two mutations that would cause the loss of one of the mutations. This approach also allowed selection of the desired colonies by simple replica plating on selective media. Firstly, two E. coli vectors were constructed in pBluescript II SK + where the wild-type S1 gene was replaced by a chloramphenicol resistance gene (CmR) (Figure (Figure1A)1A) or by a modified S1 gene including the desired mutations (Figure (Figure1B);1B); both flanked by 1.2 and 1.5 kb of the S1 upstream and downstream regions, respectively. These vectors were then processed and their inserts were introduced into pSS4245. These derivatives were transferred into E. coli SM10 for conjugative transfer and allelic exchange into B. pertussis strain Tohama. The plasmid pSS5Cm3 generated a replacement of the S1 gene by the CmR marker (Figure (Figure2A).2A). The plasmid pSS5S13-9 K-129 G restored the S1 gene into its original location, now with the two desired mutations (Figure (Figure2B).2B). After selection of isolates on selective media, integration of the CmR and modified S1 genes at the expected position was confirmed by PCR amplification (data not shown). The integration of the mutated S1 gene at the designated position was confirmed by PCR with specific primers that could hybridize the upstream 5 and 3 prime downstream flanking regions and internally in the S1 gene (data not shown). The mutations in the S1 gene of the clone selected for further manipulation was confirmed by DNA sequencing. The new strain was designated as Bp-WWC.
Initial attempts to increase PT expression by inserting the whole ptx-ptl operon into a multi-copy plasmid compatible with B. pertussis failed to deliver useful strains suggesting that the over-expression of PT is potentially toxic and must remain within certain limits to obtain viable strains. In order to increase the PT toxin yield, a second set of PT structural genes was introduced into the Bp-WWC chromosome. To identify an insertion target site, the sequence of the B. pertussis Tohama genome (accession number NC_002929) was scanned and many pseudogenes were identified. The DNA sequence (posn. 2905288) between a putative ammonium transporter gene and a putative auto-transporter gene was selected for insertion (posn. 2903988-2905228 and 2905291-2908277). These genes each carry frameshift mutations which ruin their functionality (Figure (Figure3A).3A). The general strategy outlined in the preceding section was followed. First, the E. coli vector pSKPD5Cm3 was constructed by inserting the CmR gene within the regions flanking the selected integration site (Figure (Figure3B).3B). After insertion of the sequences of interest into pSS4245, allelic exchange was selected by the CmR marker. Integration of the CmR gene at the designated position was confirmed by PCR (data not shown). In the second vector, five PT structural genes with mutated S1 were inserted between the ptx-ptl operon promoter and terminator (following the S3 gene) to generate the vector pSKptxter (Figure (Figure3C).3C). Allelic exchange into the selected target integration inserted a second copy of the functional cluster of the PT structural genes into Bp-WWC strain. The new strain was designated as Bp-WWD. This strain harboured two copies of ptx operon with mutated S1 gene. The result of integration was verified by amplification of the upstream, downstream, and internal regions of the ptx operon, that all showed the expected integration without disruption of the regions where recombination had occurred.
Automated sequencing was applied to confirm the presence of the desired mutations. In the case of strain Bp-WWD that has two integrated copies of the S1 gene, PCR amplification yields, in principle, a mix of the copies of the two genes. An unexpected point mutation in one of the inserts would appear as a double-nucleotide assignment at the corresponding position. The single peak of fluorescence signal at the R9K and E129G positions indicated the correct sequence on Bp-WWC and that of the two copies of S1 in Bp-WWD had identical mutations. The sequence around the two desired mutations is reported in Figure Figure44 that shows the sequencing records for strain Bp-WWD and the sequence alignments for wild-type Tohama, Bp-WWC and Bp-WWD.
Due to the low level of PRN expression, a second copy of the prn structural gene (under control of the 246 bp fha promoter and its own terminator) was introduced into the Bp-WWD chromosome (posn. 1345693) between the two pseudogenes of putative exported dehydrogenase (posn. 1344710-1345685) and a putative aspartate racemase (posn. 1345693-1346049) (Figure (Figure5A).5A). The pSKPD2Cm3 E. coli vector was constructed where the CmR gene was inserted between the upstream and downstream regions flanking the selected insertion site. Another vector was constructed using the same flanking regions and the prn gene under control of the fha promoter (Figure (Figure5B).5B). After insertion of the CmR marker in the desired location, the CmR gene was replaced by the prn functional block using the usual allelic-exchange selection and screening procedures.
The B. pertussis strains isolated from this construction exercise did not express PRN and the expression level of the other (FHA, PT and hemolysin) antigens was not detectable (data not shown). It was tentatively concluded that the PRN product is toxic if overproduced under control of the stronger fha promoter and only escape mutants having lost the capacity to produce PRN or all virulence factors were viable. It was, therefore, decided to introduce the natural prn promoter in place of the fha promoter. The plasmid pSKPD25FpPRN3 was used to replace the fha promoter by the original prn promoter to generate a functional cassette with its own natural promoter and terminator (Figure (Figure5C).5C). This functional cassette was inserted at the selected site by the usual allelic-exchange procedure to obtain a strain with a second non-tandemly-repeated copy of the prn gene under control of its own promoter. The expected insertion was confirmed by PCR amplification with primers binding to the flanking regions internally in the prn gene. This strain was normally viable and was designated as Bp-WWE.
The strain Bp-WWE was cultured and serially sub-cultured in Modified Stainer-Scholte (MSS) medium to reach approximately 50 generations. The last culture was diluted and plated onto MSS agar. Thirty isolated colonies were randomly picked, and analyzed for their S1 and prn genes by PCR (data not shown). The results showed that all colonies contained two copies of S1 and prn genes at the expected positions.
The production of PT and FHA in shake flask cultures was analyzed by ELISA. Shake flask cultures were all performed in MSS medium containing heptakis(2,6-O-dimethyl)β-cyclodextrin [23,24]. At 36 h, the production of PT was about doubled in strain Bp-WWD (3.77 ± 0.53 μg/mL), compared with Bp-WWC (2.61 ± 0.16 μg/mL) and wild-type Tohama (2.2 μg/mL) (Table (Table1),1), demonstrating that the level of PT expression was a function of the number of copies of the structural gene cluster. FHA in all three recombinant strains was about the same (Table (Table1).1). The production of PRN in shake flask cultures of Bp-WWC, Bp-WWD and Bp-WWE in MSS medium was analyzed by densitometry analysis of Western blot results. PRN amount in the clarified culture supernatants and extract of the separated cells at 60°C was assayed. The amount of PRN in cell extract of Bp-WWC and Bp-WWD was similar (2.48 ± 0.10 and 2.31 ± 0.17 μg/mL, respectively). A two-fold increase was found in Bp-WWE (4.18 ± 1.02 μg/mL), again showing a good correlation of the level of prn expression to the gene copy number. In all three recombinant strains, the fraction of PRN found in the supernatant fraction in these flask cultures was small or negligible (less than 0.1 μg/mL, data not shown).
PT was purified from culture supernatants using a modification of the process published by Ozcengiz  where the initial ammonium sulphate precipitation was replaced by ligand exchange chromatography [26,27]. The toxicity of the PT toxin from wild type B. pertussis and Bp-WWC (genetically inactivated PT) was analysed and compared by the Chinese hamster ovary (CHO) cell clustering assay . This assay has a much higher sensitivity than other functional assays reported for PT. The native toxin purified from strain B. pertussis Tohama demonstrated a clustering endpoint at 2.6 pg per well. The genetically-inactivated PT did not promote clustering at the highest concentrations of 0.8-1.6 μg per sample obtained in this test (Figure (Figure6).6). This assay can, therefore, detect toxicity reduction by a factor of 5 × 105 to 1 × 106, despite limitations imposed by the low solubility of PT. This result demonstrated that PT toxin purified from Bp-WWC was successfully inactivated by insertion of five nucleotide replacements resulting in two amino acid replacements in the PT subunit S1.
Unmarked gene insertion and replacement were successful, using pSS4245 as vector in B. pertussis. After a second homologous recombination to excise the plasmid, no antibiotic gene marker nor any scars were left in the chromosome when compared with the cre-lox system  or earlier allelic-exchange procedures used in Bordetella . Overproduction of genetically-deactivated PT toxin was reported in 1992  by using tandem repeats of ptx genes or another copy inserted into the fha gene. The resulting recombinant B. pertussis strain overproduced PT up to 80 mg/L. Tandemly-repeated genes are a known potential cause of genetic instability. For this reason, the genome sequence of B. pertussis was scanned to look for suitable integration sites. The DNA position between two terminators of pseudo-genes (putative ammonium transporter and putative auto-transporter genes) was selected as integration sites for the ptx cluster. The copy number for the PT structural cluster was limited to two, as overproduction of these virulence factors places a burden on cell metabolism, resulting in slower growth and potentially genetic instability, as shown by preliminary results.
Over-expression of prn gene by the fha promoter to drive higher expression was apparently toxic to growth of B. pertussis, possibly in resulting from higher PT expression. Our results showed that replacement of the prn promoter with a stronger one did not provide increased prn expression . Therefore, increasing the gene copy number under the control of the native prn promoter was the approach selected. The fha promoter of the second gene copy was replaced by the native prn promoter to generate a strain with a second copy of the prn gene and its native promoter inserted into another location on the chromosome. The toxicity of PRN to the host cell was also reported in E. coli . The fha promoter was then replaced by the native prn promoter, then the resulting strain exhibited normal growth in shake flasks and expressed twice the amount of PRN. The distribution of PRN between culture supernatant and cell extract was modified - a larger fraction of total PRN was found in the supernatant although in shake flasks, the quantities of PRN spontaneously released into the supernatant were minimal. The presence of either two copies of mutated PT gene alone or together with two copies of prn in WWC, WWD or WWE did not show any genetic instability as evidenced by serial-subculture experiment. All recombinant strains showed the presence of two copies of corresponding genes and corresponding amount of PT and PRN. Hence, homologous recombination among the homologous copies was not so far found in these strains.
Although bacterial growth in shake-flask culture is limited due to rapid pH rise and intoxication from release of ammonia by metabolism of the glutamate carbon source , shake-flask culture provides a useful indication of the strain's potential under optimized fermentor conditions. The construction of stable strains with enhanced expression of PT (Bp-WWD) or of the two limiting antigens PT and PRN (Bp-WWE) was demonstrated. With enhanced production of PT alone, Bp-WWD could not generate sufficient quantities of PRN, therefore in this case, the use of an independent supply of PRN in recombinant E. coli or P. pastoris would be required. As the expression level of both PT and PRN has been equally increased in strain Bp-WWE, it would be expected that matching quantities of the two antigens would also be obtained in higher-density cultures, thereby simplifying vaccine manufacturing operations.
B. pertussis strains that contains genetically-inactivated S1::R9K-E129G subunits of PT were constructed without leaving any markers or scars in their chromosomes. An about two-fold increase in expression of PT toxin was found in shake flasks by integrating the 5 structural genes (ptx with S1 mutated) under the control of the ptx-ptl operon promoter and terminator between two pseudo-genes on the chromosome. The presence of detoxified PT was confirmed by the CHO cell clustering assay. In addition, PRN production was increased by integration of a second copy of the prn gene between other pseudo-genes located elsewhere on the chromosome. The strains were found to be genetically stable in shake flask sub-cultures at higher generation numbers than would be required to reach large-scale fermentations (> 1,000 L). These recombinant strains, in particular, strain Bp-WWE (where the ratio of expression of PT and PRN antigens matches the composition of commercial Pertussis vaccines), should enable production of affordable acellular Pertussis vaccines. The lower Cost of Goods (CoG) is provided by the lower dose of native antigens required for adequate immunogenicity and the higher productivity the two limiting antigens PT and PRN.
All chemicals and reagents used in this study were either molecular biology or analytical grade. Chemicals were purchased from Merck (Germany) and Sigma (USA). Bacterial culture media were obtained from Difco (USA) and Merck. Restriction and modifying enzymes were purchased from New England Biolabs (USA).
E. coli DH5α (Invitrogen, USA) was used as a cloning host. This strain was grown at 37°C in Luria Bertani (LB) medium. The E. coli DH5α transformants were grown in LB medium supplemented with appropriate antibiotics: amplicillin (50 μg/mL) or chloramphenicol (15 μg/mL). E. coli SM10 and pSS4245 were obtained from Dr. Earle S. Stibitz and used as a conjugative donor strain and an allelic exchange vector, respectively. This strain was grown at 37°C in LB medium supplemented with kanamycin (50 μg/mL). The E. coli SM10 transformants were grown in LB medium supplemented with kanamycin (50 μg/mL), amplicillin (50 μg/mL) and neomycin (10 μg/mL). B. pertussis Tohama was obtained from ATCC (BAA-589). B. pertussis strains were grown at 35°C on Bordet-Gengou (BG) agar or MSS medium . One liter of the MSS medium contained 10.7 g of monosodium glutamate, 0.24 g of L-proline, 2.5 g of NaCl, 0.5 g of KH2PO4, 0.2 g of KCl, 0.1 g of MgCl2·6H2O, 0.02 g of CaCl2·2H2O, 6.1 g of Tris base, 10 g of casamino acids 0.01 g of FeSO4·7H2O, 0.04 g of L-cysteine, 0.1 g of glutathione, 0.02 g of ascorbic acid, 0.004 g of niacin and 1 g of dimethyl-β-cyclodextrin. Plasmid pBluescript II SK + and pACYC184 were obtained from Stratagene (USA) and New England Biolabs (USA), respectively.
The chromosomal DNA of B. pertussis strain Tohama was used as source material. The upstream region of the S1 gene was amplified by PCR using the 5'F-PT-SalI and 5'R-PT-MCS primers. The latter contained KpnI, XbaI, BglII and NotI sites. The amplification product was recovered from agarose gel and purified by QIAEX II Extraction kit (Qiagen, Germany). The 1287 bp amplification product was digested with SalI and NotI and cloned into the E. coli vector pSKΔKpnI digested with the same enzymes. pSKΔKpnI was a derivative of pBluescript II SK + where the KpnI site was removed by digestion, trimming 3' protruding end by the Klenow enzyme, and re-circularization. The resulting construct was transformed by heat shock into competent cells of E. coli DH5α and designated as pSK5'. The downstream region was likewise obtained by amplification with the 3'F-PT-XbaI and 3'R-PT-BglII primers. The 1531 bp product was digested with XbaI and BglII and the recovered fragment inserted into pSK5' digested with the same enzymes to obtain pSK53.
The CmR gene was obtained from plasmid pACYC184. The gene was amplified using the primers CmF-KpnI and CmR-XbaI. The 1295 bp PCR product was purified and digested with KpnI and XbaI and inserted into pSK53 cut with the same enzymes. The resulting plasmid was designated as pSK5Cm3. This plasmid incorporated the chloramphenicol resistance gene flanked by the 5'-upstream and 3'-downstream regions of the S1 gene (Figure (Figure1A1A).
To perform the allelic exchange, vector pSS4245  was used. Plasmid pSK5Cm3 was digested with SacI and BglII and the recovered fragment ligated into pSS4245 cut with SacI and BamHI. After transformation into E. coli SM10, the resulting plasmid was designated as pSS5Cm3. Fresh cultures of B. pertussis strain Tohama (4 days on MSS-agar with 20 mM nicotinic acid) and of E. coli SM10 harbouring the vector (overnight on LB-agar with ampicillin, kanamycin and chloramphenicol) were scraped and mixed onto agar plates containing LB:MSS (1:1) with 20 mM nicotinic acid and 10 mM MgCl2. After 3 h-cultivation at 35°C, the mix was swabbed onto MSS with 20 mM nicotinic acid, 50 μg/mL streptomycin and 5 μg/mL chloramphenicol. Streptomycin and chloramphenicol were used to select against E. coli SM10 (donor cell) and B. pertussis (recipient cell). The swab growth was streaked onto MSS agar with 5 μg/mL chloramphenicol for the second recombination event. The resulting single colonies were tested by replica plating and a few colonies with the SmS and CmR phenotype were retained for further testing (Figure (Figure2A).2A). The integration of CmR gene at designed position was confirmed by PCR using the primers that specifically bind to the upstream 5' (5'F-int and 5'RCM-int primers) and 3' (3'FCM-int and 3'R-int primers) downstream flanking regions and internally in the CmR gene. From the PCR analysis, it was confirmed that the 5' and 3' flanking regions were present and the CmR gene had been inserted at the expected location in place of the S1 gene. These verifications also confirmed that the allelic-exchange process had not caused any alteration in the S1 flanking regions where recombination had taken place.
The S1 gene was cloned by PCR amplification and mutated by site-directed PCR mutagenesis. The primers S1F-PT-KpnI and S1R-PT-XbaI (Table (Table2)2) were used to amplify the gene from chromosomal DNA. The purified PCR product was digested with XbaI and KpnI and the recovered 908 bp fragment was ligated into pSK53 cut with the same enzymes. After transformation and colony selection, the resulting plasmid was designated as pSK5S13.
Site-directed PCR mutagenesis used the internal F-R9K and R-R9K primers with the sequence mismatch CGC→AAG, causing the R9K substitution. The same procedure was applied to generate the second mutation using the internal mismatched primers F-E129G and R-E129G, to generate the sequence GAA→GGG, causing the E129G substitution.
The resulting fragment was digested with XbaI and KpnI and inserted into pSK53 cut with the same enzymes to obtain plasmid pSK5S13-9 K-129 G (Figure (Figure1B).1B). This was digested with SacI and BglII and the recovered fragment was ligated into pSS4245 cut with SacI and BamHI. After transformation into E. coli SM10, the resulting plasmid was designated as pSS5S13-9 K-129 G.
Allelic exchange to insert the modified S1 gene back into its original location in the B. pertussis chromosome was performed as above but without selection of the exconjugants by chloramphenicol. The desired strains in this case have lost this marker and therefore screening by replica plating was necessary to identify colonies with the desired phenotype CmS and SmS. The resulting Tohama derivative was designated as Bp-WWC (Figure (Figure2B).2B). The integration of the S1 mutated gene at the designated position was confirmed by PCR with the specific primers. The primers could bind the upstream 5' (5'F-int and R-R9K primers), 3' (F-E129G and 3'R-int primers) downstream flanking regions, and inside the S1 gene.
The sequences flanking the targeted insertion site (Figure (Figure3A)3A) were first cloned to obtain pSKPD5Cm3. The upstream 1688 bp fragment was amplified with the primers 5'F-PD-ApaI and 5'R-PD-MCS, digested with ApaI and KpnI, and ligated into pSK5Cm3 cut with the same enzymes to yield pSKPD5'-Cm. The downstream 2980 bp fragment was amplified with the primers 3'F-PD-MCS and 3'R-PD-BglII, digested with XbaI and BglII, and ligated into pSKPD5'-Cm cut with the same enzymes. The resulting plasmid was designated as pSKPD5Cm3 (Figure (Figure3B3B).
The conjugative construct was obtained by digesting this plasmid with NotI and BglII and ligation into pSS4245 which was digested with NotI and BamHI, resulting in plasmid pSSPD53-Cm. Conjugative transfer and selection for SmS and CmR provided the desired B. pertussis derivative Bp-PD53-Cm, where the presence of the intact upstream, downstream, and CmR insert was confirmed by PCR amplification. The primers could bind the upstream 5' (5'FPD-int and 5'RCM-int primers), 3' (3'FCM-int and 3'RPD-int primers) downstream flanking regions, and inside the CmR gene.
A functional copy of the ptx operon with its promoter was generated by insertion of the ptx-ptl terminator next to the S3 gene. The five structural genes of PT (modified S1, S2, S4, S5, and S3) with its operon promoter were amplified from Bp-WWC DNA using the primers PtxF-BamHI and PtxR-MCS. The 3469 bp amplified product was digested with BamHI and SpeI and the recovered fragment was ligated into pSKΔRI cut with the same enzymes to yield pSKptx. Plasmid pSKΔRI is a variant of pBluescript II SK + where the EcoRI site has been removed by digestion and filled-in with the Klenow enzyme and re-circularized.
The ptx-ptl operon terminator was then amplified with the TerF-EcoRI and TerR-SpeI primers. The 223 bp product was doubly digested with EcoRI and SpeI and ligated into pSKptx cut with the same enzymes. After transformation and colony selection, the resulting plasmid was designated as pSKptxter (Figure (Figure3C).3C). This plasmid was then doubly digested with BamHI and SpeI and ligated into pSSPD5Cm3 cut with the same enzymes to yield the conjugative vector pSSPDptxter. Allelic exchange into Bp-PD53Cm was performed as described above with replica screening for SmS and CmS colonies to obtain the strain designated as Bp-WWD. The integration of S1 mutated gene at the designated position was confirmed by PCR with specific primers. The primers could bind the upstream 5' (5'FPD-int and R-R9K primers), 3' (F-E129G and 3'RPD-int primers) downstream flanking regions, and internal S1 gene.
A derivative of pBluescript SK + lacking the BamHI site was constructed by digestion with the enzyme, filling-in with the Klenow enzyme, and ligation. The resulting plasmid was transformed into E. coli and designated as pSKΔH1.
The sequence of the B. pertussis Tohama strain was scanned and pseudo-genes were identified. The DNA sequence (posn. 1345693) between a putative exported dehydrogenase (posn. 1344710-1345685) and a putative aspartate racemase pseudo-gene (posn. 1345693-1346049) was selected as the insertion site. These two genes carried frameshift mutations and were not functional (Figure (Figure5A).5A). The 5'-upstream region to the targeted insertion site was amplified using primers carrying SpeI (5'F-PD2-SpeI) and a multilinker including BamHI and NotI (5'R-PD2-MCS) restriction sites. The amplified product was isolated by gel electrophoresis and doubly digested with SpeI and NotI. The resulting fragment was ligated into a fragment of pSKΔH1 which was digested with the same enzymes. The resulting plasmid was transformed into E. coli and designated as pSKPD25. The 3'-downstream fragment was similarly amplified with primers carrying XbaI(3'F-PD2-XbaI) and NotI (3'R-PD2-NotI) restriction sites. After digestion with the same enzymes, the resulting fragment was ligated into a fragment of pSKPD25 digested with the same enzymes. The resulting plasmid was transformed into E. coli and designated as pSKPD253.
The chloramphenicol resistance gene was obtained by PCR amplification from plasmid pACYC184 using primers carrying a BamHI(CmF-BamHI) and XbaI (CmR-XbaI) restriction site. The PCR product was digested with the two enzymes and cloned into pSKPD253 cut with the same enzymes. After ligation, the resulting plasmid was transformed into E. coli, verified by restriction analysis and designated as pSKPD25Cm3. The plasmid was digested with NotI and SpeI and the resulting fragment was ligated into pSS4245 which was doubly digested with the same enzymes. The resulting plasmid was designated as pSSP2D5Cm3 and transformed into E. coli SM10. Conjugation was conducted as described above by using Bp-WWD as the recipient B. pertussis strain with selection of CmR and SmS single colonies. The integration of CmR gene at its designated position was confirmed by PCR with the primers that specifically bind to only the upstream 5' (5'FPD2-int and 5'RCM-int primers), 3' (3'FCM-int and 3'RPD2-int primers) downstream flanking regions, and inside the CmR gene.
The structural gene of PRN was amplified from B. pertussis DNA using a primer starting at the ATG start codon (F) and a primer carrying an XbaI (R) restriction site. The 2,808 bp amplified product containing only the coding region and the terminator was treated by an 'A' tailing protocol (Promega, USA). The resulting fragment was cloned into pGEM-T easy vector to obtain a plasmid designated as pGEM-TPRN which was verified by restriction analysis. In an initial workup to create a second copy of the PRN gene driven by the stronger FHA promoter, the FHA promoter was isolated from B. pertussis DNA by PCR amplification and inserted ahead of the PRN gene. The FHA promoter was amplified by primers carrying the BamHI (FHAproF-BamHI) and a polylinker containing NdeI-XbaI (FHAR-MCS). The purified product was cut with BamHI and XbaI then the recovered DNA fragment was ligated into pSKPD253 cut with the same enzymes. The resulting plasmid designated as pSKPD253Fp was verified by restriction analysis. This plasmid was cut with NdeI and XbaI, then ligated with the PCR product of the prn gene which was amplified from pGEMTPRN by PRNF-NdeI and PRNR-XbaI primers and cut with the same enzymes. The resulting plasmid was designated as pSKPD25FpPRN3 (Figure (Figure5B).5B). The conjugative construct was obtained by digesting this plasmid with NotI and SpeI and ligation into pSS4245 digested with the same enzymes. The resulting plasmid was designated as pSSPD2FpPRN. This construct was inserted at the selected location of the Bp-WWD chromosome to replace the chloramphenicol resistance marker introduced using the usual allelic-exchange procedures and screening as described above.
The PRN promoter was cloned by PCR amplification of the B. pertussis DNA using primers with the restriction sites BamHI (PrnProF-BamHI) and NdeI (PRNProR-NdeI). The plasmid pSKPD25FpPRN3 was cut with BamHI and NdeI to generate a fragment which had lost the FHA promoter. The PRN promoter was ligated in its place. After transformation into E. coli and verification by restriction analysis, the resulting plasmid was designated as pSKPD25PRN3 (Figure (Figure5C).5C). The plasmid was cut with NotI and inserted into pSS4245 cut with the same enzyme. The resulting construct, pSSPD2prn was transferred into E. coli SM10 to conduct the allelic exchange. The resulting B. pertussis strain was designated as Bp-WWE. Integration of the prn gene at its designated position was confirmed by PCR with the primers that specifically bind only to the upstream 5' (5'FPD2-int and PRNProR-NdeI primers), 3' (PRNF-int and 3'RPD2-int primers) downstream flanking regions, and inside the prn gene.
The Bp-WWC, Bp-WWD and Bp-WWE strains were grown in shake flasks with 100 mL MSS medium supplemented with methylated β-cyclodextrin (1 g/l) at 35°C with shaking speed of 200 rpm. After 32-48 h of growth, the culture supernatants were collected and assayed by ELISA to quantify the PT and FHA expression level. As PRN releasing from its membrane-bound precursor is the result of an imprecise cleavage by unidentified proteases , PRN expression was determined by Western blot with densitometric analysis to evaluate the integrity of the antigen. This assay was conducted both on the clarified culture supernatant and the cell extract obtained by heating cell suspension in isotonic buffer (10 mM Tris-HCl pH 8.0, 150 mM NaCl, 0.002% NaN3, and 1 mM PMSF) at 60°C for 30 min and the supernatant was collected after centrifugation at 10,000 × g, 4°C for 30 min.
Purified rabbit polyclonal antibodies against PT or FHA (NLAC, Thailand) with the dilution of 1:1000 in carbonate/bicarbonate buffer (pH 9.6) were coated in 96-well plates (NUNC Maxisorp, Denmark) for 100 μL per well and incubated overnight at 4°C. After 3 time-washing with phosphate-buffered saline pH 7.4 containing 0.1% Tween 20 (PBST), blocking was performed using 100 μL per well of 3% bovine serum albumin (BSA)-PBST then incubated at 37°C for 1 h. After discarding the blocking buffer and washing, dilutions of the standard PT, FHA or samples were loaded and incubated at 37°C for 1 h. Then, anti-PT mouse monoclonal antibody (Abcam, USA) at 1:30,000 dilution or anti-FHA mouse monoclonal antibody (NIBSC, UK) at 1:10,000 dilution in blocking buffer was added and incubated under the same conditions. After washing the wells for three times with PBST, 100 μL of rabbit anti-mouse (H + L) IgG-HRP conjugate (Abcam, USA) in blocking buffer at 1:10,000 dilution was used as secondary antibody and incubated for 37°C for 1 h. After washing with PBST, 100 μL of enzyme substrate, 3,3',5,5'-tetramethylbenzidine (KPL, USA), was added. The colour reaction was terminated with 1 N HCl, 100 μL per well. Optical density was measured at 450 nm using a microtiter plate reader. ELISA assay for PT and FHA of each recombinant strain was done in three replicates using three independent cultures.
Dilutions of standard PRN and samples were resolved in a 10% SDS-PAGE gel then transferred to a PVDF membrane using a semi-dry blotting system. The membrane was blocked with 5% skim milk in PBST for 1 h. After discarding the blocking solution, the membrane was incubated with 20 mL anti-PRN sheep serum (NIBSC, UK) at 1:10,000 dilution in blocking buffer for 1 h, then washed three times with PBST. The membrane was then incubated under the same conditions with 20 mL of rabbit anti-sheep IgG-HRP conjugate (Santa Cruz Biotechnology, USA) and washed again. The membrane was then immersed in 3,3'-diaminobenzamidine until the brown colour developed. The reaction was terminated by rinsing 2-3 times with de-ionized water, then left to dry at room temperature. Western blot of PRN of the three recombinant strains was performed in three replicates using cell extracts from three independent cultures of each strain. The membranes were scanned and converted to a picture file. PRN concentrations were derived by densitometric analysis of the sample and reference bands using ImageJ software http://rsbweb.nih.gov/ij/.
The strains were cultured in 100 mL MSS medium at 35°C and agitated at 200 rpm for 48 h, then 0.1 mL of culture was transferred into 100 mL MSS and incubated under the same conditions. This step was repeated four more times. Each transfer corresponded to 50 generations. The culture was diluted and plated on MSS agar. Thirty isolated colonies of a final plating were randomly picked and analysed by PCR to detect the expected presence of ptx and prn inserts.
CHO cell clustering activity was determined by the method of Hewlett et al.  In short, CHO cells were cultured in the cRPMI 1640 medium supplemented with 10% fetal bovine serum. The cells were incubated at 37°C under 5% CO2 atmosphere. After trypsinization, 200 μL of CHO cell suspension at density of 2 × 104 cells/mL were seeded in a 96-well micro-culture plate. Test samples and reference PT toxin were serially diluted at ten-fold intervals in phosphate-buffered saline (PBS) pH 7.4 and a 25 μL volume of the dilutions was added to each well. After incubation for 48 h under the same conditions to permit maximal clustering, cells were stained with crystal violet and photographed.
PT: Pertussis toxin; PRN: Pertactin; FHA: Filamentous hemagglutinin; rPT: recombinant Pertussis toxin; ELISA: Enzyme-Linked Immunosorbent Assay
The authors declare that they have no competing interests.
WB, AL and PP conceived the study. WP, CB, AI and JP designed the experiments. WB wrote the draft of manuscript, JP and WP revised the manuscript. All authors read and approved the final version of the manuscript.
We are grateful to Dr. Earle S. Stibitz, at the Division of Bacterial, Parasitic, and Allergenic Products, Center for Biologics Evaluation and Research, Food and Drug Administration, USA, for the generous provision of pSS4245, E. coli SM10 and directions for their use for conjugative transfer and allelic exchange in Bordetella. We thank Dr. Kanchana Kenkoom, at the National Laboratory Animal Center (NLAC), Mahidol University, Thailand and Prof. Watchara Kasinrerk at the Biomedical Technology Research Unit, Chiang Mai University, Thailand, for the preparation of polyclonal and monoclonal antibodies. We acknowledge the participation of Assoc. Prof. Worawidh Wajjwaku, Department of Pathology of Veterinary Medicine, Kasetsart University, Thailand, for performing the PT toxicity tests in CHO cells. We thank Dr. Pramvadee Wongsangchandra of the Department of Biotechnology, Faculty of Science, Mahidol University, and Eiakalak Hemjinda, Greanggrai Hommalai, Kulnaree Phetrong, Nantidaporn Ruangchan, and Chutintorn Suadee of Bionet-Asia Co. Ltd., Hi-Tech Industrial Estate, Bang Pa-In, Thailand, for their participation to seeding procedures, purification of antigens and assay development.