Oral re-vaccination of Eurasian wild boar with Mycobacterium bovis BCG yields a strong protective response against challenge with a field strain

Background

Field vaccination trials with Mycobacterium bovis BCG, an attenuated mutant of M. bovis, are ongoing in Spain, where the Eurasian wild boar (Sus scrofa) is regarded as the main driver of animal tuberculosis (TB). The oral baiting strategy consists in deploying vaccine baits twice each summer, in order to gain access to a high proportion of wild boar piglets. The aim of this study was to assess the response of wild boar to re-vaccination with BCG and to subsequent challenge with an M. bovis field strain.

Results

BCG re-vaccinated wild boar showed reductions of 75.8% in lesion score and 66.9% in culture score, as compared to unvaccinated controls. Only one of nine vaccinated wild boar had a culture-confirmed lung infection, as compared to seven of eight controls. Serum antibody levels were highly variable and did not differ significantly between BCG re-vaccinated wild boar and controls. Gamma IFN levels differed significantly between BCG re-vaccinated wild boar and controls. The mRNA levels for IL-1b, C3 and MUT were significantly higher in vaccinated wild boar when compared to controls after vaccination and decreased after mycobacterial challenge.

Conclusions

Oral re-vaccination of wild boar with BCG yields a strong protective response against challenge with a field strain. Moreover, re-vaccination of wild boar with BCG is not counterproductive. These findings are relevant given that re-vaccination is likely to happen under real (field) conditions.

Wildlife vaccination is increasingly being explored as a tuberculosis (TB) control tool in all major wildlife reservoirs. An attenuated mutant of M. bovis, Mycobacterium bovis BCG (bacille Calmette Guerin [1]), is often the vaccine used in wildlife vaccination trials worldwide [2–8]. In countries such as UK and the Republic of Ireland, Eurasian badger (Meles meles) vaccination field trials are becoming part of the TB control strategies [9]. Field vaccination trials are also ongoing in Spain, where the Eurasian wild boar (Sus scrofa) is regarded as the main driver of animal TB at the wildlife-livestock interface [10–12].

In Mediterranean Spain, modeling of tuberculosis in wild boar populations predicted that over 70% of the annual cohort of wild boar piglets would be needed to be vaccinated in order to significantly reduce the prevalence of the disease and eventually eradicate the infection [13]. It has been demonstrated that the most efficient oral vaccine bait deployment strategy in this area consists in using selective piglet feeders and deploying vaccine baits both at the start (late June/early July) and the end of summer (late August/early September), in order to gain access to a high proportion of early and late born wild boar piglets respectively, avoiding the hottest period from late July to early August [14, 15]. However, with this strategy of a double delivery in summer, it would be probable that some individuals actually gain access to vaccine baits twice in a season. This possibility of some wild boar ingesting vaccine baits in both vaccination campaigns raises the question of the effects of re-vaccination in wild boar. In human beings, revaccination with BCG confers only a modest advantage over single vaccination [16, 17]. Among cattle and wildlife MTC hosts, there are controversial studies regarding the use of a single dose or the need of a booster dose of the vaccine to achieve a better vaccination protocol (Table 1). Re-vaccination has the potential to be counter-productive, and such risks needed to be assessed in wild boar as an integral part of vaccine safety. Although adverse effects of re-vaccination or over-dosage of BCG in wild boar were not expected, we were interested in assessing the effects of re-vaccination with a 52 day interval imitating field conditions.

The aim of this study was to assess the response of wild boar to re-vaccination with BCG and to subsequent challenge with an M. bovis field strain, under experimental conditions. Based on current knowledge, we expected a protective response similar to those recorded in previous single dose BCG vaccination experiments [2, 22].

Experiment design

Seventeen 3-4-month-old wild boar piglets were bought in a commercial farm known to be free of mycobacterial lesions at slaughter and with a fully negative ELISA test [23]. The animals were housed in class III bio-containment facilities with ad libitum food and water. Wild boar piglets were randomly assigned to treatment (BCG vaccinated animals) or control groups (unvaccinated animals). The M. bovis BCG Danish reference strain (CCUG 27863) was cultured on Coletsos medium (Biomerieux, France), and prepared as described for previous experiments [22]. Vaccine containing 10⁶ cfu was administered orally in baits designed for wild boar piglets [24]. For the challenge, 5 ml of a suspension containing 10⁵ colony forming units (cfu) of an M. bovis field strain were administered by the oropharyngeal route as described in previous experiments [2, 22]. The isolate used for challenge was originally isolated from a naturally infected wild boar and identified as M. bovis spoligotype profile SB0339 according to the M. bovis Spoligotype Database website (http://www.mbovis.org).

The animals were handled five times during the experiment, including vaccination (T0, day 1), re-vaccination 52 days after the first vaccination (T1, day 52), challenge 74 days after re-vaccination (T2, day 126), one blood sampling two months after challenge (T3, day 185) and necropsy four months after challenge (T4, day 255). Handling procedures and sampling frequency were designed to reduce stress and health risks for subjects, according to European (86/609) and Spanish laws (R.D. 223/1988, R.D. 1021/2005). The protocol was approved by the Committee on the Ethics of Animal Experiments of the Regional Agriculture Authority (Diputación Foral de Vizcaya, Permit Number: BFA10.373 (27/19/2010)).

Sampling, pathology and microbiology

Blood samples were collected at T0-T4 time points for RNA extraction from PBMC and serum preparation. Animals were anesthetized by intramuscular injection of Zoletil (Virbac, Esplugues de Llobregat, Spain) and euthanized by captive bolt. At necropsy, all wild boar were carefully inspected for the presence of macroscopic TB-compatible lesions. Samples for culture were immediately processed and copies frozen at -80°C for mRNA isolation. TB-compatible lesions were classified based on lesion distribution and lesion intensity, and scored as previously described [2]. Briefly, lymph nodes and the oropharyngeal tonsils were scored as 0 (No visible lesion), 1 (1–2 small (<1 cm) caseous foci), 2 (Several small foci), 3 (Same and at least one lesion >1 cm) or 4 (Diffusely affected); lung lobes were scored as 0 (No visible lesion), 1 (Few small lesions), 2 (Numerous or clustered small lesions with some coalescence), 3 (Densely clustered small lesions), 4 (Same and at least one large lesion) or 5 (Two or more large lesions). Visceral organ lesions were scored as 0 (No visible lesion), 1 (1–2 mm foci scattered throughout organ) or 2 (5–10 mm diameter clusters of 1–2 mm foci or single focus >1 cm diameter). Lymphoid tissues and samples of lung tissue were cultured for mycobacteria and scored (total number of culture-positive samples) as described in [22]. All isolates were spoligotyped in order to confirm the strain [25]. Tonsil samples were flash frozen and stored in liquid N until used for gene expression studies.

Serology and interferon tests

Serum samples were tested for anti-PPD immunoglobulin G (IgG) antibodies by means of an in-house ELISA using bovine tuberculin purified protein derivative (bovine PPD; CZ Veterinaria SL, Porriño, Lugo, Spain) as antigen and protein G horseradish peroxidase (Sigma-Aldrich, Madrid, Spain) as a conjugate applying the protocol described by Boadella et al. [23]. Serum samples were also tested by the DPP technology developed by Chembio Diagnostic Systems, Inc. using selected M. bovis antigens. Briefly, the presence and intensity of either of the 2 separate test lines (T1, MPB83 antigen; T2, CFP10/ESAT-6 fusion protein) were evaluated by a DPP optical reader (in relative light units, RLU) [23]. Blood samples taken at times 2, 3 and 4 were also used for detection of the IFN-gamma response in presence of avian and bovine PPD, as described previously [22].

RNA isolation and real time RT-PCR

Total RNA was extracted from wild boar PBMC and tonsils using TRI reagent (Sigma, Madrid, Spain) following manufacturer’s recommendations. RNA was used for real-time RT-PCR analysis of mRNA levels of selected genes in individual samples. Selected genes are involved in innate immunity (complement component 3, C3 and interleukin 1-beta, IL-1b) and methylmalonyl CoA mutase, MUT. Real-time RT-PCR was performed with gene-specific primers (C3, SsC3-L: acaaattgacccagcgtagg and SsC3-R: gcacgtccttgctgtactga; IL-1b, SsIL1beta-L: ccaaagagggacatggagaa and SsIL1beta-R: ttatatcttggcggcctttg; MUT, SsMUT-L: gtttgccaacggtgaaaagt and SsMUT-R: aatgagcttcaaggcagcat) using the One-Step RT-PCR Kit with SYBR Green and the CFX thermal cycler (Bio-Rad, Hercules, CA, USA) following manufacturer’s recommendations. Control reactions were performed using the same procedures, but without RT to monitor DNA contamination in the RNA preparations and without RNA added to monitor contamination of the PCR reaction. A dissociation curve was run at the end of RT-PCR reaction to ensure that only one amplicon was formed and that the amplicon denatured consistently at the same temperature range for every sample [26]. The mRNA values were normalized against S. scrofa cyclophilin (SsCyclophilin-L: agcactggggagaaaggatt and SsCyclophilin-R: cttggcagtgcaaatgaaaa), β-actin (Ss-BactinF: ggacctgaccgactacctca and Ss-BactinR: ggcagctcgtagctcttcat) and GAPHD (Ss-GAPHDF: gtcggttgtggatctgacct and Ss-GAPHDR: agcttgacgaagtggtcgtt) using the genNorm ddCT method [27].

No clinical signs such as wasting or cough were recorded during the experiment. Figure 1 presents the pathology scores and total culture scores. BCG re-vaccinated wild boar showed reductions of 75.8% and 66.9%, respectively, as compared to controls (U tests; Z > 3.2, p < 0.01). Two BCG re-vaccinated wild boar had no positive culture. The mean (±SE) thorax culture scores were 0.22 (±0.3) for vaccinated and 2.25 (±0.3) for control wild boar (90.2% reduction; U test; Z = 3.1, p < 0.01). Only one of nine vaccinated wild boar had a culture-confirmed lung infection, as compared to seven of eight controls (Fisher’s test; p = 0.003).

Wild boar TB lesion scores (left) and culture scores (right) at necropsy. The solid lines show the median values.

Full size image

Serum antibody levels were highly variable and did not differ significantly between BCG re-vaccinated wild boar and controls (ANOVA; Treatment effect F_{1, 45} < 2.71, p > 0.05). Gamma IFN levels differed significantly between BCG re-vaccinated wild boar and controls (ANOVA; Treatment effect F_{1, 39} = 6.08, p < 0.05). The gamma IFN response to bPPD was undetectable at T2. A peak was recorded at T3 both in BCG re-vaccinated wild boar (mean OD ± SE 6.9 ± 1.7) and in controls (11.4 ± 1.8), slightly declining in both groups thereafter (Figure 2).

Mean optical density (OD) readings of the gamma interferon ELISA in BCG re-vaccinated (solid line) and control (dashed line) wild boar. Vertical bars represent 95% confidence intervals.

Full size image

The mRNA levels for IL-1b, C3 and MUT were significantly higher in vaccinated wild boar when compared to controls at T2 and decreased after mycobacterial challenge (Figure 3A). Only IL-1b mRNA levels remained higher in vaccinated animals when compared to controls until the end of the experiments (Figure 3A). In tonsils, only MUT mRNA levels were significantly higher in vaccinated than in control animals at the end of the experiment (Figure 3B).

Gene expression in response to BCG vaccination in wild boar. The mRNA levels of selected genes were analyzed by real-time RT-PCR in (A) PBMC of vaccinated and control wild boar collected at T0 (before vaccination), T2 (before challenge) and T4 (at necropsy) or (B) tonsils at T4. The mRNA levels were normalized against S. scrofa cyclophilin, β-actin and GAPHD and normalized Ct values were represented as Ave + S.D. in arbitrary units and compared between groups by Student´s t-test with unequal variance (*P ≤ 0.05).

Full size image

This experiment confirmed that oral BCG re-vaccination of wild boar induces a strong protective response against challenge with an M. bovis field strain. This response includes lower lesion and culture scores; lower gamma IFN levels and higher IL-1b, C3 and MUT mRNA levels in vaccinated wild boar.

The main difference between this experiment and the previous vaccine and challenge trials in wild boar was re-vaccination. Although no single vaccination controls were included, the protective response recorded after re-vaccination (76% lesion score, 67% culture score), was higher than those recorded in two previous single dose BCG vaccination experiments, i.e. 56% reduction in lesion score, 50% in culture score [2]; 52% reduction in lesion score, 9% in culture score [22]. This animal experiment was run along with another one testing a new, heat-inactivated vaccine, and the number of available experimental wild boar and the available housing space did not allow including a single-vaccination BCG group. Serum antibody and gamma IFN responses were essentially similar to those recorded in these single vaccination experiments. These levels of protection were better than those documented for BCG-Pasteur re-vaccinated African buffaloes (Syncerus caffer), in which revaccination gave not differences in the protection for vaccinated animals compared to unvaccinated animals [4]. In ferrets (Mustela furo), two doses of 5×10⁸ cfu of BCG-Pasteur given orally in a 4 week interval produced a significant reduction in pathology after oral challenge with virulent M. bovis, decreasing the mean bacterial count for retropharyngeal LN tissue of culture- positive vaccinated animals to 70% [7].

It is known that factors such as the variation of the period between the administration of the two doses of the vaccine could affect the protective efficacy of the vaccination. For example, the reduction of this period from 8 to 4 weeks in vaccinated red deer did not affect the protection induced by the vaccine, whereas increasing this period to 43 weeks largely ablated protection [28]. In our study, wild boar vaccination took place 52 days after the first vaccination (between 7-8 weeks), which imitates field conditions.

Another important factor that could affect the protection of the vaccine is the dose. Low and medium booster doses (10⁴-10⁷ cfu; 6-8 weeks interval) of BCG-Pasteur produced significant protection against infection and disease in vaccinated red deer, but higher booster doses (5×10⁸cfu) provided protection against disease but not against infection [5, 18]. In our case, a dose of 10⁶ cfu was used, again imitating field protocols.

Molecular characterization of host-pathogen interactions identified wild boar genes such as MUT, C3 and other innate and adaptive immune response genes involved in resistance to mycobacterial infection [29–33]. As in previous experiments, C3 and MUT mRNA levels rose after vaccination and decreased after challenge [22]. The up-regulation of genes encoding pro-inflammatory cytokines such as pro-IL-1b probably stimulates the production of C3 which may contribute to the protective response to BCG vaccination in wild boar.

Oral re-vaccination of wild boar with BCG yields a strong protective response against challenge with a field strain. One important conclusion of this study is that re-vaccination of wild boar with BCG is not counterproductive as suggested for cattle [34]. This finding is relevant given that wild boar TB is increasingly reported [35, 36] and that re-vaccination is likely to happen in the ongoing field vaccination trials.

Carlos Martín, Universidad de Zaragoza, kindly provided the vaccine BCG strain. Many colleagues at SaBio IREC, NEIKER and VISAVET granted valuable technical help. This is a contribution to EU FP7 grant 613779 WildTBVac and to MINECO Plan Nacional grant AGL2011-30041 and FEDER.

Author notes

Affiliations

1. SaBio IREC (CSIC-UCLM-JCCM), Ronda de Toledo s/n, Ciudad Real, 13005, Spain

   • Christian Gortazar
   • , Beatriz Beltrán-Beck
   • , Mariana Boadella
   • , Ruth C Galindo
   • , Vidal Montoro
   •  & Jose de la Fuente

2. NEIKER-Tecnalia, Animal Health Department, C/Berreaga 1, Derio, Bizkaia, E-48160, Spain

   • Joseba M Garrido
   • , Iker A Sevilla
   •  & Ramón Juste

3. Departamento de Sanidad Animal, Facultad de Veterinaria, Universidad Complutense de Madrid, Avenida de Puerta de Hierro s/n, Madrid, 28040, Spain

   • Alicia Aranaz

4. Chembio Diagnostic Systems Inc., Medford, NY, 11763, USA

   • Konstantin P Lyashchenko

5. Centro de Vigilancia Sanitaria Veterinaria (VISAVET), Facultad de Veterinaria, Universidad Complutense de Madrid, Avenida de Puerta de Hierro s/n, Madrid, 28040, Spain

   • Lucas Domínguez

6. Department of Veterinary Pathobiology, Center for Veterinary Health Sciences, Oklahoma State University, Stillwater, OK, 74078, USA

   • Jose de la Fuente

Corresponding author

Correspondence to Christian Gortazar.

Competing interests

The authors declare that they have no competing interests.

Authors’ contributions

BB-B, JMG, AA, LD, RJ, JdlF and CG: contributed to the conception, design, and data collection, laboratory work, drafting and writing of the manuscript. IAS, MB, KPL, RCG and VM: contributed to laboratory work, data analysis and drafting of the manuscript. All authors have read and approved the final manuscript.

Christian Gortazar, Beatriz Beltrán-Beck contributed equally to this work.

Reprints and Permissions