Abattoir-based study on the epidemiology of caprine tuberculosis in Ethiopia using conventional and molecular tools
© Deresa et al.; licensee BioMed Central Ltd. 2013
Received: 12 May 2012
Accepted: 15 February 2013
Published: 21 February 2013
Despite the important role of goats for meat and milk production in Ethiopia, little information is available on the epidemiology of caprine tuberculosis (TB). Caprine TB is important as milk is usually consumed raw particularly by Ethiopian pastoralists. The objectives of the present study were to estimate the prevalence of TB in goats at an abattoir, to evaluate associated risk factors and to characterize the causative mycobacteria.
A cross-sectional study was conducted on 1990 randomly selected male goats that were slaughtered at Luna Export Abattoir of central Ethiopia. Postmortem examination, mycobacterial culturing and molecular typing techniques like genus typing, deletion typing and spoligotyping were used.
The overall prevalence of caprine TB-like lesions was 3.5%. The lesion prevalence increased significantly with increasing age. Mycobacteria were found by culture and seen as acid fast bacilli in 12% of the goats with TB-like lesions. Characterization of the eight isolates using multiplex polymerase chain reaction (PCR) indicated that five of them belonged to the genus Mycobacterium. Four of the latter were confirmed to be members of the M. tuberculosis complex. Further characterization of the three M. tuberculosis isolates by spoligotyping identified them as type SIT53 and two new spoligotypes.
The isolation of M. tuberculosis from goats in this study indicates a potential risk of transmission of M. tuberculosis between humans and goats.
Caprine tuberculosis (TB) caused mainly by Mycobacterium bovis and M. caprae[1, 2] poses a risk to goat health and production in developing world[3–5]. Recently, reports of caprine TB have increased in several countries; even in those practicing a long standing test and slaughter policy[2, 3, 5–10]. It is reported that the infection is widespread in Africa where goats co-graze with cattle that are not subject to TB testing and slaughter regimes[9–11]. Goats may become infected with M. bovis when sharing pastures with infected cattle, at watering points, market places and shared night shelters.
In Ethiopia, mixed farming of cattle and goats is a common practice. Livestock move freely from one region to another and from farm-to-farm. Thus, this practice poses a high risk of inter- and intraspecies transmission and spread of M. bovis infection. This mixed farming of small and large ruminants is especially a risk to goats in countries like Ethiopia where bovine TB is endemic and reports have shown a prevalence of bovine TB ranging from 3.4% in small holder production systems to 50% in intensive dairy production systems[14–17].
A previous study reported a prevalence of 4.2% TB in Ethiopian goats and also reported the occurrence of the disease for the first time in Ethiopia. However, that study did not identify the species of the M. tuberculosis complex (MTBC). Thus, there is little information on the status and etiology of caprine TB in Ethiopia. As scientific knowledge is required to design appropriate control methods, this study was performed to estimate the prevalence of caprine TB in slaughter goats, evaluate associated risk factors, and characterize the causative agents.
Materials and methods
Study site and animals
This study was conducted in Luna Modern Export Abattoir at Modjo Town, which is located 73 km southeast of Addis Ababa in central Ethiopia. The abattoir is privately owned and primarily male goats are slaughtered for export purpose.
All goats were of local breeds and originated mainly from Arsi, Borana, Jimma, Somali and South Wello representing different agro-ecological zones. All goats had been kept under extensive production systems either as mixed crop–livestock production system or as a pastoral system of production. Goats were purchased at different local markets and transported to the abattoir. At the abattoir, animals were fed, watered, and rested for 24 to 72 hrs before being slaughtered. The TB status of the goats was not known as there was no pre-slaughter tuberculin skin testing scheme.
Our project was evaluated and approved by the Institional Review Board (IRB) of the Aklilu Lemma Institute of Pathobiology, Addis Ababa University. The Reference Number of the approval letter/Minutes is IRB/01/2011-12
Study design and sampling techniques
A cross-sectional study design was used. The design involved stratification of the goats according to geographic origin and goat type to estimate the prevalence of caprine TB and assess the potential risk factors of the disease. The goat type was defined according to its origin and the physical description given earlier. The study goats were also categorized into two age groups conventionally: ≤ 1.5 years as young, and >1.5 years as adult on the basis of the dentition as described earlier for African indigenous goats.
The selection of the goats was based on systematic random sampling while the goats were moving in line to the slaughter hall. The selected goats were identified using permanent marker, kept separately after selection and released for slaughter one after the other. The sampling interval was obtained by dividing the total number of animals slaughtered from specific geographical origin within specific day by the estimated daily sample size. Twelve goats were sampled during every study day. Thus, the total number of animal slaughtered in the particular day from a particular origin was divided by twelve and every Nth animal was selected after random selection of the first animal until the daily sample size was met. Accordingly, a total of 1990 goats were examined.
Postmortem inspection was performed following a procedure described previously. All pulmonary lobes and the lymph nodes of the head (retropharyngeal, mandibular), thorax (mediastinal and bronchial), mesenterium, and liver were examined thoroughly. The carcass including internal organs and lymph nodes were examined under a bright-light source.
The lung and the lymph nodes were cut into approximately 2 cm thick slices to facilitate the detection of lesions using separate sterile scalpel blades. The cut surfaces were examined visually under bright light for the presence of lesions compatible with TB[22, 23]. Gross nodular lesions of caseous necrosis and/or calcification were considered as suspected for TB. Such tissues were collected for bacteriological culture into sterile universal bottles with 5 ml of 0.9% saline solution. The samples were transported to Aklilu Lemma Institute of Pathobiology (ALIPB) on the same day and stored at +2 to +8°C for a maximum of one month until mycobacteriological culturing was carried out. However, almost all samples were cultured within a few days of sampling.
Culturing and identification of mycobacteria
Specimen processing and culturing for mycobacteria was carried out at TB laboratory of ALIPB in accordance with the guidelines of the Office des Internationale Epizooties. In the laboratory, individual tissue specimens were sectioned using sterile blades in sterile Petri dishes to obtain fine pieces and then homogenized with a mortar and pestle. The homogenate was decontaminated using 2 ml of 4% NaOH for 15 min and then centrifuged at 3,000 rpm for 15 min. The supernatant was discarded and the sediment was neutralized by 1% (0.1 N) HCl using phenol red as indicator. Neutralisation was considered to be achieved when the color of the solution was changed from purple to yellow.
Thereafter, 0.1 ml of the suspension was inoculated onto a duplicate set of Löwenstein-Jensen (LJ) slants; one supplemented with 0.4% sodium pyruvate (LJ pyruvate) and the other with glycerol (standard LJ). Cultures were incubated aerobically at 37°C for at least eight weeks with weekly observation for growth according to. Positive cultures were confirmed by Ziehl–Neelsen staining and heat killed in water bath at 80°C for 45 min. The heat killed isolates was stored at −20°C for further molecular typing.
Mycobacterial genus typing
Primers used for genus and RD9 typing of isolated mycobacteria
Primer sequence(5′ to 3′)
396 bp (presence of RD9)
575 bp (absence of RD9)
M. tuberculosis strains (H37Rv) and M. avium were used as positive controls while Qiagen water was used as negative control. The reaction mixture was then heated in a Programme Thermal Controller (Applied Biosystem; PTC- 100™) using the following amplification programs: 95°C for 10 min for enzyme activation; 95°C for 1 min for denaturation; 61°C for 0.5 min for annealing; 72°C for 2 min for extension; involving 35 cycles all in all and final extension at 72°C for 10 min.
A 1.5% agarose gel was prepared and the products were electrophoresed in 10×TAE running buffer. Ethidium bromide at ratio of 1:10, 100 bp DNA ladder, and orange 6x loading dye were used in gel electrophoresis. Finally, bands were visualized using alpha innotech, version 126.96.36.199 (Alpha Innotech Corporation) in a multi–image™ light cabinet.
Region of difference (RD) deletion typing
For deletion typing, the procedure described earlier was followed. The RD9 deletion typing was carried out on isolates that showed band for M. tuberculosis complex by genus typing. Each sample was tested in a separate PCR tube. Primers directed against the RD9 were used to generate a deletion profile that would allow species identification of the isolate.
RD9 is a 2030 base pair (bp) gene segment of M. tuberculosis and PCR analysis using flanking primers revealed that RD9 is absent in M. bovis, M. microti, and M. africanum. Primers used for RD9 typing and the size of PCR product size expected in the presence or absence of the respective region of difference is given in Table 1.
The reaction mixture consisted of: 10 μl of HotStarTaq master mix, 0.3 μl × 3 of each primer (flank_R, F and Int) of the respective deletion typing, 2 μl DNA template and 7.1 μl Qiagen water to a final volume of 20 μl. M. tuberculosis H37Rv and M. bovis 2122/97 were used as positive controls while Qiagen water was used as negative control. The mixture was heated in a Programme Thermal Controller (Applied Biosystem; PTC- 100™) using an initial hot start of 95°C for 15 min followed by 35 cycles of 95°C for 1 min; 55°C for 1 min; and 72°C for 1 min; a final extension step of 72°C for 10 min to complete the cycle. PCR products were electrophoresed in 1.5% agarose gel in 10× TAE running buffer. Ethidium bromide at ratio of 1:10,100 bp DNA ladder and orange 6× loading dye (Gene Craft, Germany) were used in electrophoresis. Finally, bands were visualized using alpha innotech, version 188.8.131.52 (Alpha Innotech Corporation) in a multi–image™ light cabinet.
Spoligotyping was performed at ALIPB; following the procedure described earlier and according to the spoligotype kit supplier’s instructions (Ocimum Biosolutions Company, Iisselstein, The Netherlands). The direct repeat (DR) region were amplified by PCR using oligonucleotide primers derived from the DR sequence (DRa:5′-GGT TTT GGG TCT GAC GAC-3′ and DRb:5′-CCG AGA GGG GAC,GGA AAC-3′). A total volume of 25 μl of the following reaction mixture was used for the PCR: 12.5 μl of HotStarTaq master mix (Qiagen). This solution provides a final concentration of: 1.5 μM MgCl2 and 200 mM of each deoxynucleotides triphosphates, 2 μl of each primer (20 p mol each), 5 μl suspension of heat-killed cells (approximately 10 to 50 ng), and 3.5 μl distilled water. PCR amplification was performed for 15 min at 96°C and then subjected to 30 cycles of 1 min at 96°C; 1 min at 55°C, 30 sec at 72°C and a final extension at 72°C for 10 min.
The amplified products were hybridized to a set of 43 immobilized oligonucleotides, each corresponding to one of the unique spacer DNA sequences within the DR locus. After hybridization, the membrane was washed twice for 10 min in 2× SSPE (1× SSPE is 0.18 M NaCl, 10 μM NaH2PO4, and 1 μM EDTA (pH 7.7) - 0.5% sodium dodecyl sulfate at 60°C and then incubated in 1:4,000 diluted streptavidin peroxidase (Boehringer, Ingelheim Germany) for 45 to 60 min at 42°C. The membrane was washed twice for 10 min in 2× SSPE - 0.5% sodium dodecyl sulfates at 42°C and rinsed with 2× SSPE for 5 min at room temperature 20°C). Hybridizing DNA (presence or absence of the unique spacers) were detected by the enhanced chemiluminescence method (Amersham, Buckinghamshire, England) and by exposure to X-ray film (Hyperfilm ECL, Amersham), which detects light signals and thereby produces a pattern which allows for typing of isolates as specified by the manufacturer.
Data collection, management and analysis
For each individual animal examined age, goat type and geographical origin were recorded on a data sheet. Presence or absence of TB-like lesions and affected tissue(s) were recorded in database based on Microsoft® Excel for Windows 2007.
Descriptive statistics was used to estimate prevalence of TB-like lesions across the individual factors and lesion frequency in different anatomical locations. Uni-and multivariate logistic regressions were used to investigate possible associations between the prevalence and the explanatory variables. P value <0.05 and 95% confidence level were used for statistical significance. Statistical analysis was carried out using SPSS version 18.0 (SPSS Inc. Chicago, IL, USA).
Prevalence of TB-like lesions in goats and associated risk factors
Individual variables, prevalence, and univariate analysis of risk factor of tuberculosis-like lesions in slaughtered goats
No of carcasses examined
No (% positive)
Multivariate analysis of risk factor with presence of tuberculosis-like lesions in goats
No. of carcasses examined
Age of goat
1.142 - 3.096
≤ 1.5 year
Origin of goat
1.068 - 5.473
0.746 - 4.462
0.744 - 4.258
0.485 - 3.187
Distribution of pathology
Most of the TB-like lesion were observed in the thoracic cavity (lung: 22% of cases, mediastinal lymph nodes: 42%, and bronchial lymph nodes: 33%) and only 3% was observed in mesenteric and hepatic lymph nodes.
Culture and acid fast test microscopy results
Seventy-eight samples from suspected TB lesions were processed and cultured. Bacterial growth was observed in 14% (11/78) of the sowed slants of which eight were confirmed to be acid fast bacilli (AFB).
Genus identification of AFB isolates
RD9 deletion typing result
Spoligotyping of M. tuberculosis isolates
An abattoir-based epidemiological survey of caprine TB was conducted on goats originated from different regions of Ethiopia. Lesion-based prevalence was calculated and mycobacteria were characterized. Compared to the two previous studies carried out on goat TB in Ethiopia, this study was more comprehensive as the number of goats included was relatively higher, the origin and types of animals was more representatives of the reference population and advanced molecular techniques were used.
The overall lesion prevalence of 3.5% reported in this study is similar to the prevalence reported in previous studies in Ethiopia. A TB-like lesion prevalence of 4.2% in 1,536 goats was reported in a study conducted in 2005 at Modjo Modem Export Abattoir. A similar prevalence (4.3% in 1,152 goats) was recorded based on gross lesions at Helmex Export Abattoir. Likewise, a prevalence of 3.1% in 193 goats was reported in goats kept at Adami Tulu Research Center using a single intradermal tuberculin test (TST). Studies conducted in other countries have also reported similar results[3, 30].
A significantly higher prevalence of TB-like lesions in goats aged >1.5 years is in agreement with a study, which reported higher prevalence in older goats although the goats were older than 6 years in that study. Similarly, several cross sectional studies conducted on bovine TB have reported higher prevalences of TB in older cattle[11, 14, 31]. This may be explained by an age depend risk of exposure.
The prevalences of TB in goats that originated from the different zones and regions were similar indicating the overall similarity of management system and infection pressure. This finding is consistent with that of an earlier study, which reported similar prevalences in different regions of Ethiopia. A significantly higher prevalence was recorded for goats originating from the Borena area as compared to those from Somali region although the goats types were the same in both areas.
The present study showed that TB-like lesions were almost exclusively observed in the thoracic cavity of goats. A similar study has shown that 97% of the gross TB-like lesions were found in the lungs and associated lymph nodes, while lesions were only found in the thoracic cavity in Algerian goats. This indicates that goats acquire the infection mainly through the respiratory route.
The isolation of three M. tuberculosis strains was unexpected as a previous study has reported that the causative agent of caprine TB in some European countries was M. bovis[9, 11] and M. caprae in several European countries. Even recently, outbreaks of TB in goats in the United Kingdom, Italy and Portugal were reported to be caused by M. bovis[2, 5, 34]. However, M. tuberculosis has previously been isolated from goats in Nigeria. The isolation of M. tuberculosis from goats in this study is likely to be due to transmission of the bacterium from TB infected people to goats as has been suggested earlier. Transmission of M. tuberculosis from man to cattle has been reported from Slovenia and in Ethiopia; cattle owned by farmers with active TB were four times more likely to have TB than cattle owned by those farmers without active TB.
This study documented an equal low prevalence of caprine TB-like lesions across a range of eco-epidemiological settings in Ethiopia. The high prevalence of lesions in the lung and associated lymph nodes suggests that transmission of TB to goats is mainly through the respiratory route. The isolation of the SIT53 strain of M. tuberculosis from goats in this study suggests transmission from humans.
The study was financially supported by Ethiopian Ministry of Agriculture, Aklilu Lemma Institute of Pathobiology and EDUlink.
- Aranaz A, Liebana E, Gomez-Mampaso E, Galan JC, Cousins D, Ortega A, Blazquez J, Baquero F, Mateos A, Suarez G, Dominguez L: Mycobacterium tuberculosis subsp. caprae subsp. nov: A taxonomic study of a new member of theMycobacterium tuberculosis complex isolated from goats in Spain. Int J Sys Bacteriol. 1999, 49: 1263-1273. 10.1099/00207713-49-3-1263.View ArticleGoogle Scholar
- Daniel R, Evans H, Rolfe S: Outbreak of tuberculosis caused by Mycobacterium bovis in golden Guernsey goats in Great Britain. Vet Rec. 2009, 165: 335-342. 10.1136/vr.165.12.335.View ArticlePubMedGoogle Scholar
- Cadamus S, Adesokan H, Jenkins A, Van Solingen D: Mycobacterium tuberculosis and M. bovis in goats, Nigeria. Em Inf Dis. 2009, 15: 2066-2069. 10.3201/eid1512.090319.View ArticleGoogle Scholar
- Hiko A, Agga GE: First-time detection of mycobacterium species from goats in Ethiopia. Trop Anim Hlth Prod. 2010, 43: 133-139.View ArticleGoogle Scholar
- Tafess K, Dawo F, Sori T, Ameni G: Prevalence of caprine tuberculosis in Mid-Rift Valley area of Oromia, Ethiopia. Afr J Microbio Res. 2011, 5: 1473-1478.Google Scholar
- Naima S, Borna M, Bakir M, Djamel Y, Fadila B, Jacob Z, Djamel G: Tuberculosis in cattle and goats in the North of Algeria. Vet Res. 2011, 4: 100-103.Google Scholar
- Regassa A, Medhin G, Ameni G: Bovine tuberculosis is more prevalent in cattle owned by farmers with active tuberculosis in central Ethiopia. Vet J. 2008, 178: 119-125. 10.1016/j.tvjl.2007.06.019.View ArticleGoogle Scholar
- Sharpe AE, Brady CP, Johnson AJ, Byrne W, Kenny K, Costello E: Concurrent outbreak of tuberculosis and caseous lymphadenitis in a goat herd. Vet Rec. 2010, 166: 591-592. 10.1136/vr.b4825.View ArticlePubMedGoogle Scholar
- Prodinger WM, Brandstätter A, Naumann L, Pacciarini M, Kubica T, Boschiroli ML, Aranaz A, Nagy G, Cvetnic Z, Ocepek M, Skrypnyk A, Erler W, Niemann S, Pavlik I, Moser I: Characterization of Mycobacterium caprae isolates from Europe by mycobacterium interspersed repetitive unit genotyping. J Clin Microbiol. 2005, 43: 4984-4992. 10.1128/JCM.43.10.4984-4992.2005.PubMed CentralView ArticlePubMedGoogle Scholar
- Nigussie T: Preliminary study of tuberculosis in small ruminants slaughtered at helimex export abattoir. 2005, Debre-Zeit, Ethiopia: DVM thesis Faculty of Veterinary MedicineGoogle Scholar
- O’Reilly LM, Daborn CJ: The epidemiology of Mycobacterium bovis infections in animals and man: a review. Tuber Lung Dis. 1995, 76: 1-46.View ArticlePubMedGoogle Scholar
- Ameni G, Desta F, Firdessa R: Molecular typing of Mycobacterium bovis isolated from tuberculosis lesions of cattle in north eastern Ethiopia. Vet Rec. 2010, 167: 138-141. 10.1136/vr.b4881.View ArticlePubMedGoogle Scholar
- Hailemariam S: A brief analysis of activities of meat inspection and quarantine division. 1975, Addis Ababa, Ethiopia: Department of Veterinary Service, Ministry of AgricultureGoogle Scholar
- Ameni G, Aseffa A, Engers H, Young D, Gordon S, Hewinson G, Vordemieier M: High prevalence and increased severity of pathology of bovine tuberculosis in Holsteins compared to zebu breeds under field cattle husbandry in central Ethiopia. ClinVac Immunol. 2007, 14: 1356-1361.Google Scholar
- Ameni G, Ragassa A, Kassa T, Medhin G: Survey on bovine tuberculosis and its public health implications to cattle raising families in Wolaita Soddo, Southern Ethiopia. Ethiop J. Anim Prod. 2001, 1: 55-62.Google Scholar
- Berg S, Firdessa R, Habtamu M, Gadisa E, Mengistu A, Yamuah L, Ameni G, Vordermeier M, Robertson BD, Smith NH, Engers H, Young D, Hewinson RG, Aseffa A, Gordon SV: The burden of mycobacterial disease in Ethiopian cattle: implication for public health. PLoS One. 2009, 4: e5068-e5070. 10.1371/journal.pone.0005068.PubMed CentralView ArticlePubMedGoogle Scholar
- Tsegaye W, Aseffa A, Machec A, Mengist Y, Bergd S, Ameni G: Conventional and molecular epidemiology of bovine tuberculosis in dairy farms in Addis Ababa City, the capital of Ethiopia. Int J Appl Res Vet Med. 2010, 8: 143-151.Google Scholar
- International Livestock Research Institute (ILRI): Goat types of Ethiopia and Eritrea: physical description and management system. 1996, Nairobi, Kenya: FARM-AfricaGoogle Scholar
- Steele M: Goats. Tropical Agriculturist and Technical Center for Agricultural and Rural Co-operation. 1996, London: Macmillan education Ltd, 120-125.Google Scholar
- Thrusfield M: Survey. Veterinary Epidemiology. 2005, Blackwell Science Ltd, 228-242.Google Scholar
- Corner LA: Post-mortem diagnosis of Mycobacterium bovis infection in cattle. Vet Microbiol. 1994, 40: 53-63. 10.1016/0378-1135(94)90046-9.View ArticlePubMedGoogle Scholar
- Asseged B, Woldesenbet Z, Yimer E, Lemma E: Evaluation of abattoir inspection for the diagnosis of M. bovis infection in cattle at Addis Ababa Abattoir. Trop Anim Hlth Prod. 2004, 36: 537-546.View ArticleGoogle Scholar
- Gracy JF: Meat Hygiene. 1986, London: Bailliere-TindallGoogle Scholar
- OIE: Bovine tuberculosis. Manual of Diagnostic Tests and Vaccines for Terrestrial Part 2, Section 2.3. Chapter 2.3.3. 2010, World Organization for Animal Health,http://www.oie.int/international-standard…/terrestrial-manual/access-online,Google Scholar
- McIlroy SG, Neill SD, McCracken RM: Pulmonary lesions and Mycobacterium. bovis excretion from the respiratory tract of tuberculin reacting cattle. Vet Rec. 1986, 118: 718-721. 10.1136/vr.118.26.718.View ArticlePubMedGoogle Scholar
- Wilton S, Cousins D: Detection and identification of multiple mycobacterial pathogens by DNA amplification in a single tube. PCR Methods Appl. 1992, 1: 269-273. 10.1101/gr.1.4.269.View ArticlePubMedGoogle Scholar
- Gordon SV, Brosch R, Billaut T, Garnier K, Eiglmeier , Cole ST: Identification of variable regions in the genomes of tubercle bacilli using bacterial artificial chromosome arrays. Mol Microbiol. 1999, 32: 643-655. 10.1046/j.1365-2958.1999.01383.x.View ArticlePubMedGoogle Scholar
- Kamerbeek J, Schouls L, Kolk A, Van Agterveld M, Van Soolingen D, Kuijper S, Bunschoten A, Molhuizen H, Shaw R, Goyal M, Van Embden J: Simultaneous detection and strain differentiation of Mycobacterium tuberculosis for diagnosis and epidemiology. J Clin Microbiol. 1997, 35: 907-914.PubMed CentralPubMedGoogle Scholar
- Crawshaw T, Daniel R, Clifton-Hadley R, Clark J, Evans H, Rolfe S, de la Rua Domenech R: TB in goats caused by Mycobacterium bovis. Vet Rec. 2008, 163: 127-132.View ArticlePubMedGoogle Scholar
- Javed MT, Ahmad L, Irfan M, Ali I, Khan A, Wasiq M, Farooqi FA, Latif MS, Cagiola M: Hematological and serum protein values in tuberculin reactor and non-reactor water buffaloes, cattle, sheep and goats. Pak Vet J. 2010, 30: 100-104.Google Scholar
- Biffa D, Inangolet F, Oloya J, Asseged B, Badaso M, Yilkal A, Skjerve E: Prevalence of bovine tuberculosis in Ethiopian slaughter cattle based on post-mortem examination. Trop Anim Hlth Prod. 2009, 41: 755-765. 10.1007/s11250-008-9248-9.View ArticleGoogle Scholar
- Vordermeier HM, Chambers MA, Cockle PJ, Whelan AO, Simmons J, Hewinson RG: Correlation of ESAT-6-specific gamma interferon with pathology in cattle following Mycobacterium bovis BCG vaccination against experimental bovine tuberculosis. Infect Immunol. 2002, 70: 3026-3032. 10.1128/IAI.70.6.3026-3032.2002.View ArticleGoogle Scholar
- Ayele WY, Neill SD, Zinsstag J, Pavlik I: Bovine tuberculosis: an old disease but a new threat to Africa. Int J Tub Lung Dis. 2004, 8: 924-937.Google Scholar
- Quintas H, Reis J, Pires I, Alegria N: Tuberculosis in goats. Vet Rec. 2010, 166: 437-438.View ArticlePubMedGoogle Scholar
- Ocepek M, Pate M, Olnir-Dovc M, Poljak M: Transmission of Mycobacterium tuberculosis from human to cattle. J Clin Microbiol. 2005, 43: 3555-3557. 10.1128/JCM.43.7.3555-3557.2005.PubMed CentralView ArticlePubMedGoogle Scholar
This article is published under license to BioMed Central Ltd. This is an Open Access article distributed under the terms of the Creative Commons Attribution License (http://creativecommons.org/licenses/by/2.0), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.