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Characterization of some Brucella species from Zimbabwe by biochemical profiling and AMOS-PCR



Bovine brucellosis caused by Brucella abortus is endemic in most large commercial and smallholder cattle farms of Zimbabwe, while brucellosis in other domestic animals is rare. The diagnosis of brucellosis is mainly accomplished using serological tests. However, some Brucella spp. have been isolated from clinical cases in the field and kept in culture collection but their biochemical profiles were not documented. We report biochemical profiling and AMOS-PCR characterization of some of these field isolates of Brucella originating from both commercial and smallholder cattle farming sectors of Zimbabwe.


Fourteen isolates of Brucella from culture collection were typed using biochemical profiles, agglutination by monospecific antisera, susceptibility to Brucella-specific bacteriophages and by AMOS-PCR that amplifies species- specific IS711. The results of the biochemical profiles for B. abortus biovar 1 (11 isolates) and biovar 2 (2 isolates) were consistent with those of reference strains. A single isolate from a goat originating from a smallholder mixed animal farm was identified as B. melitensis biovar 1. The AMOS-PCR produced DNA products of sizes 498 bp and 731 bp for B. abortus (biovar 1 and 2) and B. melitensis biovar 1, respectively.


We concluded that the biochemical profiles and AMOS-PCR characterization were consistent with their respective species and biovars. B. abortus biovar 1 is likely to be the predominant cause of brucellosis in both commercial and smallholder cattle farms in Zimbabwe.


The Brucellae are small Gram-negative coccobacilli bacteria affecting both animals and humans [1, 2]. There are nine recognized species; B. abortus, B. melitensis, B. suis, B. canis, B. ovis, B. neotomae, B. ceti, B. pinnipedialis and B. microti [35]. On the basis of phenotypic profiles, some Brucella spp. are further divided into biovars [3].

Studies of the genome of Brucella spp. have demonstrated the existence of more than 70% homology [6] and based on DNA-DNA hybridisation, a single species, B. melitensis was once proposed, with the other species being biovars [7]. However, the traditional classification into nine different species is still used. This has been further supported by the recent discovery of B. ceti and B. pinnipedialis from marine mammals [5], or B. microti from a common vole Microtus arvalis [4]. The genomic similarity makes the differentiation of Brucella spp. difficult, and often a study of biological and physiological characteristics is required [3].

In Zimbabwe, only B. abortus and B. melitensis have been reported to cause animal brucellosis. B. melitensis infection was confirmed in a goat flock, believed to have been translocated from Mozambique [8, 9]. Brucellosis in wildlife has been demonstrated by serology [10] and in one instance B. abortus was isolated from a Cape buffalo (Syncerus caffer) [11]. Bovine brucellosis is a problem in some commercial dairy cattle farms, while others have eradicated [12]. Previous studies showed higher seroprevelance of between 10-53% in commercial herds in different regions of the country compared to 0-16% in communal (smallholder) cattle [9, 12]. The disease continued to be closely monitored by the use of the milk ring test (MRT), serological surveys and bacteriological investigations [1214]. Consequently, from 1988 to 2006, Brucella spp. isolates have been collected from infected herds from different parts of the country and kept in our laboratories. Although some these isolates have been identified to the species level, the details of their biochemical profiles and biovars have not been documented. The aim of this study was to characterize all Brucella field isolates in our culture collection that originated from both commercial and smallholder cattle farms of Zimbabwe using biochemical profiles and polymerase chain reaction (AMOS-PCR). The PCR assay is based on the repetitive genetic element, the insertion sequence 711 (IS711), that is unique to Brucella spp. For most Brucella spp., multiple copies of the IS711 occur at a unique species or biovar-specific chromosomal locus [15].

Materials and methods

The details of the identity and origin of all the Brucella spp. isolates, including the reference strains, used in this study are listed in Table 1. Prior to use, all strains from culture collection were stored either as lyophilized or in a -80°C deep freezer. Lyophilized isolates were re-constituted and cultured in tryptone soya broth (TSB) (Oxoid) and subsequently sub-cultured onto Farrell's medium (Oxoid) and assessed for purity on bovine blood agar (Oxoid). All plates were incubated at 37°C under 10% CO2. Isolates were then inoculated into TSB with 5% glycerol, frozen and exported to Norway for further characterization.

Table 1 Brucella isolates used in the study and the details of their geographical regions of origin.

For the observation of colonial morphology, Brucella spp. isolates were cultured on Mueller-Hinton agar (Oxoid) and single colonies were examined using a low power stereoscopic microscope illuminated by obliquely reflected light as described [3]. The tests for production of urease, catalase, oxidase, H2S and indole; sensitivity to dyes (thionin and basic fuchsin) were carried out as described by Alton and co-workers [3]. Further tests for CO2 requirement, sensitivity to dyes, lysis by bacteriophages (Tbilisi, Tb; Berkeley, Bk2; Firenze, Fi; Izatnagar, Iz1; R/C) and agglutination by A, M and R monospecific antisera were carried out at the Central Veterinary Laboratory, UK, using the procedures described [3].

The Brucella spp. isolates were grown on Farrell's agar (Oxoid) and incubated for 48 hours at 37°C under 10% CO2. To yield DNA, a few colonies from a pure culture were harvested and suspended in 200 μl of sterile distilled water in Ependorf tubes. A homogeneous suspension was made by stirring with the inoculation loop. Bacterial cells were inactivated by heating the tubes at 100°C for 10 minutes on a heating block (Grant Instruments, UK). To separate the DNA, killed bacterial cells were centrifuged at 15, 700 × g for 10 minutes. The supernatant containing crude DNA template was pipetted into new sterile Ependorf tubes and the sediment discarded. The concentration of the extracted crude DNA was measured using a ND-1000 V3.0 spectrophotometer (NanoDrop® Technologies Inc., USA). The DNA was stored at -20°C until further tests were carried out.

The AMOS-PCR (B. a bortus, B. m elitensis, B. o vis and B. s uis- Polymerase Chain Reaction) was done as described previously [15] but with minor modifications of the assay environment. Briefly, PCR assay reaction mixture consisted of the following: 1 × PCR buffer (Applied Biosystems), 3 mM MgCl2, 200 μM (each) of the four deoxynucleotide triphosphates (dNTPs) (Finnzymes Oy, Espoo, Finland), and the 5 sets of primers (0.2 μM each) of B. abortus, B. melitensis, B. ovis, B. suis and IS711-specific primer. One and half units (1.5 U) of AmpliTaq Gold® DNA polymerase (Applied Biosystems) per 45 μl reaction mixture was added and then dispensed into MicroAmp vials (Applied Biosystems). A total of 5 μl DNA template of killed bacteria (estimated at 200 ng/ml) was added per 45 μl reaction mixture. The PCR was performed with a PTC-200 Peltier Thermocycler (Roche Molecular Systems Inc, Almelda, USA). Amplification was performed for 35 cycles, each cycle comprised of denaturation at 95°C for 1 minute and 15 seconds, annealing at 60°C for 2 minutes, and extension at 72°C for 2 minutes. The PCR products were incubated for a further 5 minutes at 72°C to allow elongation of products before storage at 4°C. The PCR products were separated by electrophoresis using 1.5% agarose gel (w/v) (BDH Electran®) at 100 V for 1.5 hours. Gels were stained with ethidium bromide and photographed using a gene snap camera (Syngene Pvt Ltd, UK).


All 14 Brucella spp. isolates characterized in this study (Table 1) yielded the following results that are typical of the genus; Gram-negative coccobacilli, non-motile, positive for modified Ziehl-Neelsen staining, oxidase and catalase production, and negative for indole production (Table 2). Their growth on Mueller-Hinton agar produced colonies that were convex, with entire edges and a smooth shiny consistency. The morphological, growth characteristics and biochemical profiles of the field isolates were similar to their respective reference Brucella species and biovars (data not shown).

Table 2 Basic biochemical and metabolic profiles of field Brucella spp. from Zimbabwe.

Isolates belonging to the same biovars showed consistently similar results, except for their CO2-dependence for growth (Table 3). Regardless of the biovar type, seven of the 13 B. abortus isolates were CO2-independent, while the remaining six strains were CO2-dependent. The B. abortus isolates were lysed by phages Tb, Fi, Bk2, Iz1 and resistant to R/C. Only one isolate was lysed by the R/C phage. The single B. melitensis isolate was resistant to all phages but showed partial lysis to Bk2 (Table 3). B. abortus isolates were agglutinated by A-antiserum and B. melitensis by the M-antiserum, but all were not agglutinated by the R-antiserum (data not shown). Eleven and two of the 13 B. abortus isolates were identified to be biovars 1 and 2, respectively (Table 3).

Table 3 Summary of phenotypic characteristics of the field Brucella spp. from Zimbabwea

The Brucella isolates were detected by the AMOS-PCR and produced predicted amplicons of sizes 498 bp and 731 bp for B. abortus and B. melitensis, respectively. Similar DNA products were produced for the reference B. abortus biovar 1 and B. melitensis biovar 1, respectively.


This paper provides the first detailed biochemical profiling and AMOS-PCR characterization of some Brucella spp. isolates from Zimbabwe. The phage sensitivity patterns of all the Brucella spp. isolates were consistent with what has been reported [16]. However, a single isolate of B. abortus (B15) was lysed by R/C phage and this susceptibility could be indicative of the presence of phage attachment sites which are present in the non-smooth phases of brucellae [16]. The B. melitensis (B10) also showed an atypical reaction because it was not lysed by the Iz1 phage which normally lyses smooth strains of this species. However, the examination of single colonies on microscopy by Henry illumination [3] showed no sign of dissociation and none of the isolates were agglutinated by the R-monospecific antiserum which is an indicator of dissociation. The agglutination reaction by monospecific antisera showed the predominance of A-specific and M-specific epitopes in our B. abortus and the B. melitensis isolate, respectively. All smooth strains of Brucella may possess either the A, M or both A and M antigenic epitopes on the O chains of the lipopolysaccharides [16].

Although phage typing is used primarily for identification at the nomen species level, some Brucella strains, especially B. melitensis may show deviation from the standard pattern of susceptibility to Bk2, Iz1 and Wb phages [16]. The use of phage typing as a means of differentiating Brucella spp. has become less discriminatory as a typing tool because of the discovery of new strains with atypical sensitivity patterns [17].

The growth characteristics and the biochemical profiles of the field Brucella spp. isolates (Table 2) were similar to those of the reference strains used in this study. In addition, the results were consistent with what is reported for Brucella spp. and biovars [2, 3, 16]. However, the requirement for CO2 for growth was at variance with reports from literature [3]. Although most strains of B. abortus biovars 1-4 require CO2 for primary isolation, this attribute is quickly lost on repeated subcultures and such isolates will adapt to growing in atmospheres without CO2 [3, 16].

The use of the AMOS-PCR results were consistent with those reported elsewhere [15]. These results confirmed the identity of the Brucella spp. that was obtained using biochemical profiles. The IS711 analysis using AMOS-PCR can identify only three B. abortus biovars, 1, 2 and 4; all three biovars of B. melitensis; biovar 1 of B. suis and B. ovis, but the individual biovars within a species are not differentiated [15]. Therefore, further DNA fingerprinting methods such as the variable number of tandem repeat analysis (VNTR) [15] could be used to investigate the molecular epidemiology of these Brucella isolates.

Although the B. abortus used in this study originated from five of the eight geographical provinces of Zimbabwe (Table 1), it is difficult to conclude on the spatial distribution due to the limited number of isolates used. These isolates could possibly be restricted to one or a few geographical regions of Zimbabwe from where they have spread through movement of infected cattle. A study of more isolates is required to determine the spatial distribution of B. abortus in Zimbabwe. However, the predominance of B. abortus biovar 1 over biovar 2 suggested that it is the major cause of bovine brucellosis in both commercial and smallholder cattle farms. Another study which used fewer Brucella isolates from commercial dairy farms reported similar findings [12]. Although B. abortus biovar 2 was also detected and originating from both the commercial and smallholder cattle farms, its distribution could be limited to a few isolated areas. Elsewhere in South Africa biovar 1 had been reported to account for about 90% while biovar 2 contributed 10% of all the B. abortus isolates [18]. South Africa, to a large extent, shares similar geographic, climatic and livestock husbandry systems with Zimbabwe. While it is difficult to explain the reasons for the distribution of these B. abortus biovars in the cattle farming sectors, this could largely be influenced by movement of infected cattle between farms. Some farms often purchase cattle from other farms for the purpose of improving the genetics of their herds [9] or in the case of smallholder farms, to restock their herds which are continuously lost due to infectious diseases and lack of adequate grazing, especially during the drought seasons.

Despite the relatively few isolates studied, our results suggested that B. abortus biovar 3 and indeed other biovars may be rare in Zimbabwe, but this requires further study. B. abortus biovar 3 has been infrequently reported in South Africa, East and North Africa, while there seems to be no reports of isolation of the other biovars [2, 18]. World wide, in countries where bovine brucellosis is endemic, B. abortus biovar 1 is predominant and B. abortus biovar 2 occurs less frequently while the other biovars are rare [2, 18].


We concluded that the biochemical profiles and AMOS-PCR characterization were consistent with their respective species and biovars. B. abortus biovar 1 is likely to be the predominant cause of brucellosis in both commercial and smallholder cattle farms in Zimbabwe. Further studies are required that will apply DNA-fingerprinting to study distribution patterns of B. abortus biovars in Zimbabwe.



B. a bortus, B. m elitensis, B. ovis, B. s uis- Polymerase Chain reaction


base pairs


deoxyribonucleic acid.


  1. WHO/FAO: Brucellosis in humans and animals, World Health Organization and Food and Agricultural Organization, 20 Avenue Appia, 1211 Geneva, Switzerland. 2006, 1-66.

    Google Scholar 

  2. Quinn PJ, Carter ME, Markey B, Carter GR: Clinical Veterinary Microbiology, Mosby International Limited, Edinburgh. 1999, 261-267.

    Google Scholar 

  3. Alton G, Jones LM, Angus RD, Verger JM: Techniques for the brucellosis laboratory, Institut National de la Recherche Agronomique, Paris, France. 1988

    Google Scholar 

  4. Scholz HC, Hubalek Z, Sedla ek I, Vergnaud G, Tomaso H, Al Dahouk S, Melzer F, Kampfer P, Neubauer H, Cloeckaert A, Maquart M, Zygmunt MS, Whatmore AM, Falsen E, Bahn P, Göllner C, Pfeffer MB, Huber B, Busse H, Nöckler K: Brucella microti sp. nov., isolated from the common vole Microtus arvalis. Int J Syst Evol Microbiol. 2008, 58: 375-382. 10.1099/ijs.0.65356-0.

    Article  CAS  PubMed  Google Scholar 

  5. Foster G, Osterman BS, Godfroid J, Jacques I, Cloeckaert A: Brucella ceti sp. nov. and Brucella pinnipedialis sp. nov. for Brucella strains with cetaceans and seals as their preferred hosts. Int J Syst Evol Microbiol. 2007, 57: 2688-2693. 10.1099/ijs.0.65269-0.

    Article  CAS  PubMed  Google Scholar 

  6. Clavareau C, Wellemans V, Walravens K, Tryland M, Verger JM, Grayon M, Cloeckaert A, Letesson JJ, Godfroid J: Phenotypic and molecular characterization of a Brucella strain isolated from a minke whale (Balaenoptera acutorostrata). Vet Microbiol. 1998, 144: 3267-3273.

    Article  CAS  Google Scholar 

  7. Verger JM, Grimont F, Grimont PAD, Grayson M: Brucella, a monospecific genus as shown by deoxyribonucleic acid hybridization. Int J Syst Bacteriol. 1985, 35: 292-295.

    Article  Google Scholar 

  8. Madzima WM: Zimbabwe: Bovine brucellosis and brucellosis of small ruminants: Diagnosis, control and vaccination. Technical series. 1987, Paris, France: Office International des Epizoties

    Google Scholar 

  9. Madsen M: The current status of brucellosis in Zimbabwe. Zimbabwe Veterinary Journal. 1989, 20: 133-145.

    Google Scholar 

  10. Madsen M, Anderson EC: Serologic survey of Zimbabwean wildlife for brucellosis. J Zoo Wildlife Med. 1995, 26 (2): 240-245.

    Google Scholar 

  11. Condy JB, Vickers DB: Brucellosis in Rhodesian Wildlife. Journal of the South African Veterinary Association. 1972, 43: 175-179.

    CAS  PubMed  Google Scholar 

  12. Mohan K, Makaya PV, Muvavarirwa P, Matope G, Mahembe E, Pawandiwa A: Brucellosis surveillance and control in Zimbabwe: bacteriological and serological investigation in dairy herds. Onderstepoort Journal of Veterinary Research. 1996, 63: 47-51.

    CAS  PubMed  Google Scholar 

  13. Manley FH: Brucellosis in Rhodesia. A report to the Director of Veterinary Services. 1969, Department of Veterinary Services, Harare, Zimbabwe

    Google Scholar 

  14. Swanepoel R, Blackburn NK, Lander KP: The occurrence, diagnosis and control of Brucellosis in cattle in Rhodesia. Rhodesia (Zimbabwe) Veterinary Journal. 1976, 7: 24-31.

    Google Scholar 

  15. Bricker BJ, Halling SM: Differentiation of Brucella abortus bv. 1, 2, and 4, Brucella melitensis, Brucella ovis, and Brucella suis bv. 1 by PCR. J ClinMicrobiol. 1994, 32: 2660-2666.

    CAS  Google Scholar 

  16. Garritty GM, Bell JA, Lilburn T: Family III, Brucellaceae Breed, Murray and Smith 1957, 394 AL. Bergey's Manual of Systematic Bacteriology. Edited by: Brenner DJ, Krieg NR, Staley JT. 2005, Springer Science and Business Media, Inc., New York, NY 10013, USA, II: 370-392. 2

    Google Scholar 

  17. Jahans KL, Foster G, Broughton ES: The characterisation of Brucella strains isolated from marine mammals. Vet Microbiol. 1997, 57: 373-382. 10.1016/S0378-1135(97)00118-1.

    Article  CAS  PubMed  Google Scholar 

  18. Bishop GC, Bosman PP, Herr S: Bovine Brucellosis. Infectious Diseases of Livestock with special reference to Southern Africa II. Edited by: Coetzer JAW, Thomson GR, Tustin RC. 1994, Cape Town: Oxford University Press, 1053-1066.

    Google Scholar 

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This study was fully sponsored by the Norwegian Council for Higher Education and Development (NUFU), project vote: pro/2002/06. We are grateful to the members of staff at the National Veterinary Institute, Oslo, for their technical assistance and in particular Dr. Arve Lund for his material support and encouragement. Our sincere appreciation goes to Ms L. Perret of Central Veterinary Laboratory, Weybridge, the UK, for further typing of the Brucella isolates.

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Correspondence to John Bwalya Muma.

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Authors' contributions

GM: Principal investigator, conceived the study, and participated in the design of the proposal, collection of Brucella isolates and culture, phenotypic and molecular characterization of isolates, analysis of results and drafting the manuscript. EB: Supervision of Brucella isolate collection, participated in phenotypic and molecular characterization of isolates, result interpretation and helped in drafting of the manuscript. JB: Participated in the design of the study, molecular characterization of isolates, result interpretation and drafting of the manuscript. ES: Participated in the design, acquisition of funds and general coordination and helped to draft manuscript. BD: Participated in phenotypic and molecular characterization of isolates, result interpretation, supervision of laboratory work and helped in drafting of the manuscript. All authors have read and approved the final manuscript.

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Matope, G., Bhebhe, E., Muma, J.B. et al. Characterization of some Brucella species from Zimbabwe by biochemical profiling and AMOS-PCR. BMC Res Notes 2, 261 (2009).

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