- Open Access
Infection and exposure to vector-borne pathogens in rural dogs and their ticks, Uganda
Parasites & Vectors volume 8, Article number: 306 (2015)
In rural parts of Africa, dogs live in close association with humans and livestock, roam freely, and usually do not receive prophylactic measures. Thus, they are a source of infectious disease for humans and for wildlife such as protected carnivores. In 2011, an epidemiological study was carried out around three conservation areas in Uganda to detect the presence and determine the prevalence of vector-borne pathogens in rural dogs and associated ticks to evaluate the risk that these pathogens pose to humans and wildlife.
Serum samples (n = 105), blood smears (n = 43) and blood preserved on FTA cards (n = 38) and ticks (58 monospecific pools of Haemaphysalis leachi and Rhipicephalus praetextatus including 312 ticks from 52 dogs) were collected from dogs. Dog sera were tested by indirect immunofluorescence to detect the presence of antibodies against Rickettsia conorii and Ehrlichia canis. Antibodies against R. conorii were also examined by indirect enzyme immunoassay. Real time PCR for the detection of Rickettsia spp., Anaplasmataceae, Bartonella spp. and Babesia spp. was performed in DNA extracted from FTA cards and ticks.
99 % of the dogs were seropositive to Rickettsia spp. and 29.5 % to Ehrlichia spp. Molecular analyses revealed that 7.8 % of the blood samples were infected with Babesia rossi, and all were negative for Rickettsia spp. and Ehrlichia spp. Ticks were infected with Rickettsia sp. (18.9 %), including R. conorii and R. massiliae; Ehrlichia sp. (18.9 %), including E. chaffeensis and Anaplasma platys; and B. rossi (1.7 %). Bartonella spp. was not detected in any of the blood or tick samples.
This study confirms the presence of previously undetected vector-borne pathogens of humans and animals in East Africa. We recommend that dog owners in rural Uganda be advised to protect their animals against ectoparasites to prevent the transmission of pathogens to humans and wildlife.
Domestic dogs live in close association with humans and livestock. At a global scale, one of the main implications of this relationship is the transmission of zoonotic diseases , with dogs participating in the transmission of over 60 zoonoses . Traditionally, households in Africa keep dogs for hunting, herding, security, and guarding livestock and scaring off vermin in nearby protected areas . In Uganda, like elsewhere in East Africa, most rural dogs roam freely. This behavior exposes them to pathogens from consuming garbage, rodents and carcasses and through inhalation during scent communication. In addition, dogs receive no prophylactic measures such as vaccinations. Indeed, a recent study demonstrated a high seroprevalence to important human and animal pathogens in Ugandan dogs, including rabies virus, canine distemper virus, parvovirus, Leishmania donovani and Toxoplasma gondii . The principal routes of transmission of zoonotic infection from dogs to humans are bites, ingestion of fecal material and arthropod vectors . On the other hand, ticks are the most important vectors of disease-causing pathogens in domestic and wild animals . Tick-transmitted infections are an emerging problem in dogs and have recently become a major focus of interest in areas of the world in which they have traditionally been considered non-endemic. This relates to both their significance to canine health, and to the possible reservoir status of the dog of potentially zoonotic disease . In addition, untreated animals like the rural dogs studied here can serve as sentinels for tick infestation in the environment and for pathogen diversity in the tick population, and pathogen incidence in the dog population can reflect pathogen infection pressure .
Dogs are carriers of tick-borne rickettsioses, which are important emerging vector-borne infections of humans worldwide, including in sub-Saharan Africa [8–10]. Six tick-borne spotted fever group pathogenic rickettsiae are known to occur in sub-Saharan Africa: Rickettsia conorii conorii, the agent of Mediterranean spotted fever; R. c. caspia, the agent of Astrakhan fever; R. africae, the agent of African tick-bite fever; and R. aeschlimannii, R. sibirica mongolitimonae and R. massiliae . In Uganda, Socolovschi et al.  detected R. conorii in Haemaphysalis punctaleachi ticks collected from a dog in Kampala. This pathogen was also detected in H. leachi in Zimbabwe . Dogs can also be infected by members of Anaplasmataceae, which are rickettsial organisms that infect human and animal leukocytes . Agents such as Ehrlichia chaffeensis and E. ewingii cause human infections of varying severity, and are considered to be emerging tick-borne zoonoses . In Cameroon, E. chaffeensis was detected in ticks from dogs in one kennel  and sequences similar to E. chaffeensis, E. canis and E. ewingii were detected in ticks from Mali and Niger .
Other vector-borne bacteria with potentially serious clinical implications are those belonging to the genus Bartonella . At present, more than 20 species or subspecies of Bartonella have been described and 12 of these are recognized as zoonotic human pathogens . Bartonella spp. has been detected in different mammal species in sub-Saharan Africa. In Nigeria, high prevalence of infection with Bartonella spp. was reported in commensal rodents and associated ectoparasites (ticks, fleas and mites), whereas in Zimbabwe, B. henselae was isolated from a captive cheetah [19, 20]. Finally, parasites belonging to the genus Babesia are protozoa found in domestic animals and are transmitted by ticks. Babesiosis is particularly severe in naïve animals introduced into endemic areas. In Africa, epidemiological studies of canine babesiosis using molecular methods have been carried out only in South Africa, Sudan and Nigeria, where B. rossi and B. vogeli were shown to be present [21–23].
The aim of this work was to detect exposure to selected vector-borne pathogens in rural dogs and associated ticks in Uganda, determine their prevalence, and characterize the implicated pathogens using molecular methods.
Dogs were sampled in 2011 during a rabies vaccination campaign in and near three conservation areas in southwestern Uganda: Bwindi Impenetrable National Park (BI), Mgahinga Gorilla National Park (MG), and Queen Elizabeth National Park (QE) (Fig. 1). BI and MG are located on the rim of the Rift Valley. These two parks host some of the most biologically diverse tropical forest in East Africa and are home to more than half of the world’s remaining mountain gorillas (Gorilla beringei beringei). QE includes a diversity of habitats, including savannah, wetlands and lowland forests, and is home to populations of protected carnivores and ungulates. These parks lie within a densely populated rural landscape; in some areas, the human population is as high as 500 people/km2, and is highest around BI. This has led to high levels of interaction between local communities and their domestic animals and local wildlife .
Two hundred and fifty-one dogs were sampled for when voluntarily brought in by their owners. Blood was obtained from the cephalic vein of 105 dogs: 91 dogs were adults (more than 12 months old) and 14 were young (between 6 and 12 months old). Blood was collected in serum separator tubes and allowed to clot, and then centrifuged at 50 g for 15 min. The serum was removed and cryopreserved in liquid nitrogen until arrival at the laboratory, where it was frozen at −20 °C. Thirty-eight blood samples were applied (100 μl) to FTA™ Nucleic Acid Collection Cards (Whatman, Maidstone, Kent, UK), air dried, and stored in sealed plastic bags until further processing.
A total of 430 ticks were collected from 101 dogs and stored in 95 % ethanol until arrival at the laboratory (Table 3). The identification of tick species was performed using the keys and descriptions in Walker et al. . After identification, ticks were preserved at −20 °C until DNA extraction. Retrieved ticks belonged to the following species: Haemaphysalis leachi, Rhipicephalus praetextatus, R. sanguineus sensu lato, R. aff. turanicus  and Amblyomma variegatum. Of these, a total of 312 ticks were selected from 52 dogs for molecular detection of tick-borne pathogens: 253 adult H. leachi, 31 adult R. praetextatus and 28 Rhipicephalus spp. nymphs. These ticks were grouped in 58 pools according to species and tested for the presence of DNA from Rickettsia spp., Anaplasmataceae, Bartonella spp. and Babesia spp. In addition, 37 fleas were retrieved from 20 dogs and identified based on their morphological characteristics according to the systematic manual of Beaucournu and Launay .
Sera were analyzed by two different techniques. Indirect immunofluorescence assay (IFA) was applied using commercial kits to detect the presence of antibodies against R. conorii (Rickettsia conorii IFA IgG Antibody kit, Fuller Laboratories, Fullerton, CA, USA) and E. canis (Ehrlichia canis IFA IgG Antibody kit, Fuller Laboratories, Fullerton, CA, USA) as described by the manufacturer. The serum samples were screened at a 1:80 or 1:50 dilution in a phosphate-buffered saline (pH 7.2) for R. conorii and E. canis assays, respectively. FITC rabbit anti-canine immunoglobulin G conjugates were used as the secondary antibodies. Reactive antibodies were then detected using a fluorescence light microscope (DM LS2, Leica Microsystems, Wetzlar, Germany) at a wavelength of 490 nm. Antibodies against R. conorii were also examined by indirect enzyme immunoassay using the Canine R. conorii EIA IgG Antibody Kit (Fuller Laboratories, Fullerton, CA, USA) according to the manufacturer’s instructions. Dog sera were diluted 1:100 and incubated in the coated microwells to allow binding of serum antibody to the solid-phase antigens (R. conorii outer membrane protein rOmpB). The microwells were then washed to remove unreacted serum proteins and a peroxidase - labelled anti-canine IgG was added to label the bound antibody. After 30 min of incubation at room temperature, the microwells were washed to remove unbound conjugate. The enzyme substrate tetramethylbenzidine (TMB) was then added to quantitate the bound peroxidase activity of the conjugate. After the addition of a stop solution, the absorbance was measured at a wavelength of 450 nm on a microtiter plate reader (Mod 680, Biorad, Hercules, CA, USA).
DNA extraction from FTA cards
From each FTA Card, the genomic DNA was extracted following the manufacturer’s instructions with minor modifications. Three punches of each FTA Card measuring 1.2-mm in diameter were used. Punches were washed three times with 100 μl of FTA Purification Reagent, followed by two washing steps with 100 μl of TE-1 Buffer (10 mM Tris–HCl, 0.1 mM EDTA, pH 8.0) and incubated for three minutes at room temperature. Discs were left at room temperature and then used directly as a template in PCR. To ensure that the extraction protocol from ticks and FTA™ Cards was appropriate and could be used in the PCR amplification for hemoparasites, the eukaryotic 18S RNA Pre-Developed TaqMan Assay Reagents (AB, Life Technologies) were used, demonstrating that a negative result corresponded to truly negative samples rather than to a problem with the DNA extraction, sample degradation or PCR inhibition.
DNA extraction from ticks
For DNA extraction, ticks were washed with PBS and left overnight in PBS at 4 °C to eliminate ethanol. The DNA was isolated from tick pools by using the High Pure PCR template preparation kit (Roche, Mannheim, Germany) according to the manufacturer’s instructions with some modifications from Solano-Gallego et al. . The samples were collected in 2 mL sterile microtubes containing 10 sterile microbeads of 1 mm diameter and 1 microbead of 4 mm diameter and 200 μL of tissue lysis buffer. The tubes were shaken with a TissueLyser (Qiagen) for 2 cycles of 1 min 30 s at a frequency of 25  and incubated overnight at 65 °C with 40 μl of proteinase K.
Real time PCR
Real time PCR of Rickettsia spp., Anaplasmataceae, Bartonella spp. and Babesia spp., were carried out in a final volume of 20 μl using FastStart Universal SYBR Green Master (Roche), 4 μl of diluted DNA (1/10 for ticks and 1/2 for blood from FTA Cards) and a final primer concentration depending on the pathogen amplified (Table 1). The thermal cycling profile was 50 °C 2 min and 95 °C 10 min followed by 40 cycles of 95 °C 15 s and 60 °C 1 min and a dissociation curve at the end of the run to assess PCR specificity. The targets amplified for each pathogen and the primers used are shown in Table 1. Water (Water Molecular Biology Reagent®, Sigma) was used as a PCR negative control and positive controls were obtained from commercial slides coated with cells infected with the pathogens or commercial DNA (MegaScreen® FLUOEHRLICHIA c., MegaScreen® FLUOBABESIA canis, MegaScreen® FLUORICKETTSIA ri., MegaScreen® BARTONELLA h. from Megacor). A nested PCR was performed with the samples that gave a positive result for Anaplasmataceae and the product of this PCR was sequenced. A subset of seven samples positive for Rickettsia spp. were further characterized by conventional PCR, amplifying several target genes using the primers described in Fernández de Mera et al. .
For species identification, positive samples were characterized at the species level by sequencing the product of the real-time PCR with the exception of Babesia spp., which was directly sequenced when possible (i.e., sufficient parasitemia present). Sequences were performed with the BigDye Terminator Cycle Sequencing Ready Reaction Kit (AB, Life Technologies) following the manufacturer’s instructions using the same primers. A region of the 18S rRNA-piroplasmid was amplified for Babesia identification . Sequences obtained were compared with those in the GenBank database (www.ncbi.nlm.nih.gov/BLAST).
The new Rickettsia sequences were submitted to the EMBL database under accession numbers LM999913-LM999916 and to the GenBank under accession numbers KR181962-KR181977.
Morphological blood analysis
Air-dried and stained smears (Diff-Quick®, QCA S.A.) from 43 dogs were examined thoroughly by light microscopy (Nikon Eclipse 50i®). Erythrocyte structure was examined to evaluate cell morphology and shape as well as the presence of abnormal cells, nucleated erythrocytes and erythrocyte agglutination. Leukocyte and platelet counts were estimated according to procedures previously described in the literature . Differential leukocyte count was done by identifying 200 consecutive leukocytes. Morphology and abnormal changes for these two cell lines were also studied. Blood films were examined to check for the presence of infectious agents and intracellular inclusions.
Age and sex-related differences in dog seroprevalence and differences in the pathogen prevalence in dogs and ticks depending on the study area were tested using Fisher’s exact tests or Chi-square tests using R (R Development Core Team, 2012).
All dogs but one were seropositive to Rickettsia spp. antibodies (99.1 %; 95 % Confidence Intervals = 94.8 %-99.9 %) and 29.5 % (95 % C.I. = 21 %-39.2 %) were seropositive to Ehrlichia spp. antibodies (Tables 2 and 3). No statistically significant differences in Rickettsia spp. seroprevalence between areas were found (in all cases, Fisher’s p > 0.05). However, Ehrlichia spp. antibodies were more frequently detected in dogs in BI (44.6 %, 95 % C.I. = 31.3 %-58.5 %) than in QE (14.8 %, 95 % C.I. = 4.2 %-33.7 %; Fisher’s p = 0.007) and MG (9.1 %, 95 % C.I. = 1.1 %-29.2 %; Fisher’s p = 0.003). No age or sex-related differences were detected in seroprevalences.
Molecular detection in dogs
From the 38 blood samples preserved on FTA cards, three dogs were infected with B. rossi (7.8 %, 95 % Confidence Intervals = 1.6 %-21.4 %): two in BI (10 %, 95% CI = 1.2 %-31.7 %) and one in QE (8.3 %, 95% CI = 0.2 %-38.5), without significant differences in prevalence between study areas, or sex and age groups. All blood samples were negative for Rickettsia spp., Anaplasmataceae and Bartonella spp.
No relevant pathological changes were observed in the blood smears. Mild anemia (11.6 % of the dogs), thrombocytopenia (11.6 %), and rouleaux (9.3 %) were the most significant findings in the analyzed smears. Intraerythrocytic piroplasms morphologically compatible with large babesiae were observed in one dog, whereas Hepatozoon gamontes were found in a second one.
Tick and flea infestation
Overall, 40.2 % (95 % CI = 34.4 %-46.9 %) of the examined dogs were parasitized by ticks. We did not retrieve all the ticks observed in the field due to practical limitations, so no data on tick abundance can be provided. Nevertheless, H. leachi was the most prevalent species in all of the study areas, representing almost 70 % of the retrieved ticks (Table 4). Fleas were identified as Ctenocephalides felis (76 % of the fleas), Echidnophaga gallinacea (16 %) and Pulex irritans (11 %). No prevalence data is provided because dogs were not systematically searched for fleas.
Prevalence of pathogens in ticks
DNA of Rickettsia spp. was detected in 18.9 % (95 % C.I. = 9.9 %-31.4 %) of the analyzed tick pools, including ten pools of H. leachi and one pool of R. praetextatus. Of the seven cases further characterized, two were confirmed as R. conorii conorii, and two as R. massiliae. Similarly, DNA of Anaplasmataceae was detected in 18.9 % (95 % C.I. = 9.9 %-31.4 %) of tick pools, including ten pools of H. leachi and one pool of R. praetextatus. One of these cases showed 99 % identity with E. chaffeensis (GenBank: CP007480.1) and one showed 99 % with Anaplasma platys (GenBank JX112780.1). Babesia rossi was detected in one pool of H. leachi (1.7 %, 95 % C.I. = 0.0 %-9.2 %) (Tables 2, 3 and 5). Unfortunately, no blood samples were obtained from this dog to determine its infection status, though piroplasms morphologically compatible with Babesia spp. were observed in its blood smear. Bartonella spp. DNA not detected in any tick pools. Three tick pools were co-infected: two with Anaplasmataceae and Rickettsia spp. and one with Anaplasmataceae and B. rossi. All Rhipicephalus spp. pools were negative.
No statistically significant differences in the prevalence of pathogens in ticks were observed between study areas and no differences in pathogen prevalence were detected between H. leachi and R. praetextatus pools.
In the present survey, we show that rural dogs in Uganda are widely exposed to some tick-borne pathogens. We also demonstrate the presence of DNA from important human and animal disease agents in both dogs and associated ticks. We provide molecular evidence of the presence of Rickettsia spp. (including the zoonotic R. conorii conorii and R. massiliae), Anaplasmataceae (including E. chaffeensis and Anaplasma platys), and B rossi. As far as we know, this study constitutes the first report of E. chaffeensis and B. rossi in dogs from Uganda or elsewhere in East Africa.
We found that almost all the analyzed dogs were seropositive to Rickettsia spp. antibodies. To the best of our knowledge, this is the highest seroprevalence to this pathogen reported in a rural dog population. We are not aware of other similar studies in African dogs. In Spain, a high seroprevalence of 82 % was also observed . In humans, Ndip et al.  reported R. africae antibodies in 26.9 % of the studied population in Cameroon using an IFA. In addition, we found that nearly one in every five tick pools were infected by this agent, also representing a higher prevalence than that reported in similar studies throughout Africa. For example, Socolovschi et al.  detected only one positive case out of 57 analyzed ticks from dogs in Kampala. Parola et al.  detected Rickettsial DNA in 7.2 % of ticks from dogs examined in Niger, Mali, Burundi and Sudan, whereas Kamani et al.  reported a prevalence of 10.5 % in ticks from dogs in Nigeria.
Near one third of the dogs included in the present study were seropositive to Ehrlichia spp. antibodies. This seroprevalence is higher than that detected in Maasai Mara, Kenya (15.5 % by IFA; ) but lower than that reported by Woodroffe et al. , who detected a seroprevalence of 86 % by IFA in rural dogs in northern Kenya. Reasons for the higher detected seroprevalence in BI are unknown and require further research. We also detected that 18.9 % of the analyzed tick pools were positive to Ehrlichia spp. We were able to confirm that at least one of the pools corresponded to E. chaffeensis and, to our knowledge, this is the first detection of this zoonotic bacterium in Uganda. A study in Cameroon detected a prevalence of 56 % of E. chaffeensis in 63 ticks collected from five dogs from one kennel . Previous studies have shown that Ehrlichia species probable emerging human pathogens in sub-Saharan Africa (reviewed in ). The detection for the first time of E. chaffeensis in Uganda has important implications in public health in this country.
Babesia rossi was identified in three dogs and in one tick pool in our survey. The prevalence in our study was nevertheless lower than that in a study carried out in Nigeria by Matjila et al. , where 65 % of the pools were infected and the majority of Babesia-infected dogs (41 %) were only infested with H. leachi. Similarly, in our study, as much as 69 % of the dogs were parasitized by this tick species. Babesia rossi is considered a natural parasite of indigenous African canids in South Africa [38, 39] and is known to be the most pathogenic for dogs among the three subspecies of B. canis, frequently causing a fatal infection despite intensive treatment . It has also been noted that Babesia infection can have devastating effects in populations of wild carnivores .
No Bartonella infections were confirmed in dogs or ticks in our study. In contrast, infection with Bartonella spp. has been described in different mammals in Nigeria, Zimbabwe and Kenya [19, 20]. However, it has to be considered that Bartonella spp. are difficult to detect in blood due to a low concentration of bacteria , and it has been recommended to culture blood before molecular probes, technique that increases Bartonella detection in dog blood .
This study confirms that previously undetected vector-borne pathogens of humans and animals are present in Uganda. Detection and identification of zoonotic pathogens is useful for improving diagnosis and applying more specific treatments, and the dog can be a useful sentinel in this regard. Our study also confirmed the importance of analyzing ticks to determine the distribution of tick-borne pathogens in the canine population in Uganda. The interaction of dogs with wildlife and the role they play in the transmission of disease is well known [35, 43]. When dogs live in close association with wildlife (in or near national parks, as in this study) it is imperative to advise dog owners to protect their animals against ectoparasites to prevent the transmission of pathogens such as B. rossi to protected carnivores. We strongly recommend the continuation of the monitoring of the studied pathogens in Uganda due to their importance in human, dog and wildlife health.
Baker P, Soulsbury C, Lossa G, Harris S. Domestic cat (Felis catus) and domestic dog (Canis familiaris). In: Gehrt SD, Riley SPD, Cypher BL, editors. Urban carnivores: ecology, conflict, and conservation. Baltimore: Johns Hopkins University Press; 2010. p. 157–72.
Macpherson C, Meslin F, Wandeler A. Dogs zoonoses and public health. Wallingfor: St George’s University; 2000.
WHO/WSPA. Guidelines for Dog population management. Geneva: World Health Organization/World Society for the Protection of Animals (WHO/Zoon/90.165); 1990.
Millán J, Chirife AD, Kalema-Zikusoka G, Cabezón O, Muro J, Marco I, et al. Serosurvey of dogs for human, livestock, and wildlife pathogens, Uganda. Emerg Infect Dis. 2013;19:680–2.
De la Fuente J, Estrada-Pena A, Venzal JM, Kocan KM, Sonenshine DE. Overview: ticks as vectors of pathogens that cause disease in humans and animals. Front Biosci. 2008;13:6938–46.
Shaw SE, Day MJ, Birtles RJ, Breitschwerdt EB. Tick-borne infectious diseases of dogs. Trends Parasitol. 2001;17:74–80.
Dantas-Torres F, Chomel BB, Otranto D. Ticks and tick-borne diseases: a one health perspective. Trends Parasitol. 2012;28:437–46.
Raoult DVR. Rickettsioses as paradigms of new or emerging infectious diseases. Clin Microbiol Rev. 1997;10:694–719.
Parola P, Paddock CD, Raoult D. Tick-borne rickettsioses around the world: emerging diseases challenging old concepts. Clin Microbiol Rev. 2005;18:719–56.
Parola P. Rickettsioses in sub-Saharan Africa. Ann N Y Acad Sci. 2006;1078:42–7.
Socolovschi C, Matsumoto K, Lou MJ, Davoust B, Raoult D, Parola P. Identification of Rickettsiae, Uganda and Djibouti. Emerg Infect Dis. 2007;13:1508–9.
Kelly PJ, Mason PR. Serological typing of spotted fever group Rickettsia isolates from Zimbabwe. J Clin Microbiol. 1990;28:2302–4.
Dvorak G, Rovid-Spickler A, Roth J. Technical fact sheets for zoonotic diseases of companion animals. In: Center for Food Security and Public Health, editor. Handbook for zoonotic diseases of companion animals. Iowa: UC of VM; 2008. p. 63–267.
Walker DH. Tick-transmitted infectious diseases in the United States. Annu Rev Public Health. 1998;19:237–69.
Ndip LM, Ndip RN, Esemu SN, Walker DH, McBride JW. Predominance of Ehrlichia chaffeensis in Rhipicephalus sanguineus ticks from kennel-confined dogs in Limbe, Cameroon. Exp Appl Acarol. 2010;50:163–8.
Parola P, Inokuma H, Camicas JL, Brouqui P, Raoult D. Detection and identification of spotted fever group Rickettsiae and Ehrlichiae in African ticks. Emerg Infect Dis. 2001;7:1014–7.
Blanco JR, Raoult D. Enfermedades producidas por Bartonella spp. Enferm Infecc Microbiol Clin. 2005;23:313–20.
Márquez FJ, Millán J, Rodríguez-Liébana JJ, García-Egea I, Muniain MA. Detection and identification of Bartonella sp. in fleas from carnivorous mammals in Andalusia, Spain. Med Vet Entomol. 2009;23:393–8.
Kamani J, Morick D, Mumcuoglu KY, Harrus S. Prevalence and diversity of bartonella species in commensal rodents and ectoparasites from Nigeria, West Africa. PLoS Negl Trop Dis. 2013;7.
Kelly P, Rooney J, Marston E, Jones D, Regnery R. Bartonella henselae isolated from cats in Zimbabwe. Lancet. 1998;351:1706.
Matjila PT, Penzhorn BL, Bekker CPJ, Nijhof AM, Jongejan F. Confirmation of occurrence of Babesia canis vogeli in domestic dogs in South Africa. Vet Parasitol. 2004;122:119–25.
Oyamada M, Davoust B, Boni M, Dereure J, Bucheton B, Hammad A, et al. Detection of Babesia canis rossi, B. canis vogeli, and Hepatozoon canis in dogs in a village of eastern Sudan by using a screening PCR and sequencing methodologies. Clin Diagn Lab Immunol. 2005;12:1343–6.
Sasaki M, Omobowale O, Tozuka M, Ohta K, Matsuu A, Nottidge HO, et al. Molecular survey of Babesia canis in dogs in Nigeria. J Vet Med Sci. 2007;69:1191–3.
Walker A, Bouattour A, Camicas J, Estrada-peña A, Horak I, Latif A, et al. Ticks of domestic animals in Africa: a guide to identification of species. Bioscience Reports: The University of Wisconsin; 2003.
Dantas-Torres F, Latrofa MS, Annoscia G, Giannelli A, Parisi A, Otranto D. Morphological and genetic diversity of Rhipicephalus sanguineus sensu lato from the New and Old Worlds. Parasit Vectors. 2013;6:213.
Beaucournu JC, Launay H. les Puces de France et du Bassin méditerranéen occidenta. In: Naturelles F française des S de S, editor. Faune de France 76. Paris: French Federation of Natural Sciences; 1990.
Solano-Gallego L, Rossi L, Scroccaro AM, Montarsi F, Caldin M, Furlanello T, et al. Detection of Leishmania infantum DNA mainly in Rhipicephalus sanguineus male ticks removed from dogs living in endemic areas of canine leishmaniosis. Parasit Vectors. 2012;5:98.
Halos L, Jamal T, Vial L, Maillard R, Suau A, Le Menache A, et al. Determination of an efficient and reliable method for DNA extraction from ticks. Vet Res. 2004;35:709–13.
de Mera IG F, Ruiz-Fons F, de la Fuente G, Mangold AJ, Gortázar C, de la Fuente J. Spotted fever group rickettsiae in questing ticks, central Spain. Emerg Infect Dis. 2013;19:1163–5.
Tabar MD, Altet L, Francino O, Sánchez A, Ferrer L, Roura X. Vector-borne infections in cats: molecular study in Barcelona area (Spain). Vet Parasitol. 2008;151:332–6.
Meyer D, Harvey J. Hematology procedures. Vet Clin Pathol. 2004;33:14–26.
Roura X, Breitschwerdt E, Lloret A, Ferrer L. Serological evidence of exposure to species in healthy or leishmania infantum -infected dogs from Barcelona, Spain. J Appl Res Vet Med. 2005;3:129–37.
Ndip LM, Biswas HH, Nfonsam LE, LeBreton M, Ndip RN, Bissong MA, et al. Risk factors for African tick-bite fever in rural central Africa. Am J Trop Med Hyg. 2011;84:608–13.
Alexander KA, Conrad PA, Gardner IA, Parish C, Appel M, Levy MG, et al. Serologic survey for selected microbial pathogens in African wild dogs (lycaon pictus) and sympatric domestic dogs (canis familiaris) in Maasai Mara, Kenya. J Zoo Wildl Med. 1993;24:140–4.
Woodroffe R, Prager KC, Munson L, Conradp A, Dubovi EJ, MazetJa K. Contact with domestic dogs increases pathogen exposure in endangered African wild dogs (Lycaon pictus). PLoS One. 2012;7(1):e30099.
Esemu SN, Ndip LM, Ndip RN. Ehrlichia species, probable emerging human pathogens in sub-Saharan Africa: environmental exacerbation. Rev Environ Health. 2011;26:269–79.
Matjila PT, Leisewitz AL, Jongejan F, Penzhorn BL. Molecular detection of tick-borne protozoal and ehrlichial infections in domestic dogs in South Africa. Vet Parasitol. 2008;155:152–7.
Uilenberg G. Babesia-a historical overview. Vet Parasitol. 2006;138:3–10.
Penzhorn BL. Why is Southern African canine babesiosis so virulent? an evolutionary perspective. Parasit Vectors. 2011;4:51.
Munson L, Terio KA, Kock R, Mlengeya T, Roelke ME, Dubovi E, et al. Climate extremes promote fatal co-infections during canine distemper epidemics in African lions. PLoS One. 2008;3:5–10.
Breitschwerdt EB, Kordick DL. Bartonella infection in animals: carriership, reservoir potential, pathogenicity, and zoonotic potential for human infection. Clin Microbiol Rev. 2000;428–438.
Pérez C, Maggi RG, Diniz PPVP, Breitschwerdt EB. Molecular and serological diagnosis of Bartonella infection in 61 dogs from the United States. J Vet Intern Med. 2011;25:805–10.
Roelke-Parker ME, Munson L, Packer C, Kock R, Cleaveland S, Carpenter M, et al. A canine distemper virus epidemic in Serengeti lions (Panthera leo). Nature. 1996;381(6578):172.
Maggi RG, Breitschwerdt EB. Potential limitations of the 16S-23S rRNA intergenic region for molecular detection of Bartonella species. J Clin Microbiol. 2005;43:1171–6.
Gil H, García-Esteban C, Barandika JF, Peig J, Toledo A, Escudero R, et al. Variability of bartonella genotypes among small mammals in Spain. Appl Environ Microbiol. 2010;76(24):8062–70.
This study received partial support from the project CGL2010-17931. We thank S. Rubanga, A. Kateregga, and all of the staff of Conservation through Public Health; the Mgahinga Community Development Organization; M. Esau; District Veterinary Officers from Kanungu, Kasese, and Kisoro local governments; V. Ticó and I. Marco for help with field work; F. Ruiz-Fons and M. Gómez for their advice during tick and flea identification, respectively; and L. Serrano for laboratory assistance. The field work was carried out in Uganda and the laboratory work at the Universitat Autònoma de Barcelona, Bellaterra, Spain.
The authors declare that they have no competing interests.
TP identified the ticks, carried out the molecular analyses and drafted the manuscript. GK, JMu and LM coordinated fieldwork and collected samples. AC collected samples. LA carried out the molecular analyses and the sequence alignment. LS, IF, EB, AP and VB performed laboratory analyses. JF and SC contributed reagents and drafted the manuscript. JMi conceived the study, collected samples and drafted the manuscript. All authors commented on, improved, and approved the final manuscript.
About this article
Cite this article
Proboste, T., Kalema-Zikusoka, G., Altet, L. et al. Infection and exposure to vector-borne pathogens in rural dogs and their ticks, Uganda. Parasites Vectors 8, 306 (2015). https://doi.org/10.1186/s13071-015-0919-x
- East Africa
- Tick-borne pathogens