The burden of leptospirosis in humans and animals in Africa is higher than that reported from other parts of the world. However, the disease is not routinely diagnosed in the continent. One of major factors limiting diagnosis is the poor availability of live isolates of locally circulating Leptospira serovars for inclusion in the antigen panel of the gold standard microscopic agglutination test (MAT) for detecting antibodies against leptospirosis. To gain insight in Leptospira serovars and their natural hosts occurring in Tanzania, concomitantly enabling the improvement of the MAT by inclusion of fresh local isolates, a total of 52 Leptospira isolates were obtained from fresh urine and kidney homogenates, collected between 1996 and 2006 from small mammals, cattle and pigs. Isolates were identified by serogrouping, cross agglutination absorption test (CAAT), and molecular typing. Common Leptospira serovars with their respective animal hosts were: Sokoine (cattle and rodents); Kenya (rodents and shrews); Mwogolo (rodents); Lora (rodents); Qunjian (rodent); serogroup Grippotyphosa (cattle); and an unknown serogroup from pigs. Inclusion of local serovars particularly serovar Sokoine in MAT revealed a 10-fold increase in leptospirosis prevalence in Tanzania from 1.9% to 16.9% in rodents and 0.26% to 10.75% in humans. This indicates that local serovars are useful for diagnosis of human and animal leptospirosis in Tanzania and other African countries.
Leptospirosis disease is widespread in humans and broad range of animal species in Africa. However, leptospirosis is highly neglected and not extensively taught in both medical and veterinary schools almost across Africa. Availability of live leptospires isolated from Africa for use in its diagnosis by the gold standard microscopic agglutination test (MAT) is also a major problem. This study reports on local Leptospira serovars and their natural hosts consisting of different animal species, for inclusion in diagnosis of leptospirosis in Africa. A total of 52 Leptospira isolates were obtained from fresh urine and kidneys. African giant pouched rats (Cricetomys sp.) and insectivore shrew species (Crocidura sp.) had the highest leptospires isolation success. These were identified by serogrouping, cross-agglutination absorption test and molecular typing. Common Leptospira serovars with their respective animals were: serovar Sokoine (cattle and rodents); Kenya (rodents and shrews); Mwogolo (rodents); Lora (rodents); Canicola (rodents); Grippotyphosa (cattle); and an unknown serogroup from pigs. Inclusion of local serovar Sokoine in serodiagnosis revealed a 10-fold increase in leptospirosis prevalence from 1.9% to 16.9% in rodents and 0.26% to 10.75% in humans. Future serodiagnosis of leptospirosis in Africa should include these serovars and serovar Hardjo, Hebdomadis, Pomona and other local isolates.
Citation: Mgode GF, Machang’u RS, Mhamphi GG, Katakweba A, Mulungu LS, Durnez L, et al. (2015) Leptospira Serovars for Diagnosis of Leptospirosis in Humans and Animals in Africa: Common Leptospira Isolates and Reservoir Hosts. PLoS Negl Trop Dis 9(12): e0004251. https://doi.org/10.1371/journal.pntd.0004251
Editor: Jakob Zinsstag, Swiss Tropical and Public Health Institute, SWITZERLAND
Received: May 23, 2015; Accepted: October 29, 2015; Published: December 1, 2015
Copyright: © 2015 Mgode et al. This is an open access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited
Data Availability: All relevant data are within the paper and its Supporting Information files.
Funding: This research was supported by grants from NUFFIC (The Netherlands) through NFP fellowship granted to GFM, funding from the Flemish Inter-university Council (VLIR) (Belgium), the European Union (Ratzooman Project, INCO-Dev ICA4-CT-2002-10056 and StopRats Project EDF FED 2013-330-223), COSTECH (Tanzania) and the International Foundation for Science (IFS: D-4666-2). The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
Leptospirosis is an understudied zoonotic disease in Tanzania and across Africa. Limited reports show a high prevalence of leptospirosis in animals and humans with Africa presenting a major burden globally . The highest median annual incidence of leptospirosis is in Africa standing at 95.5 per 100,000 people. Africa is followed by Western Pacific (66.4), the Americas (12.5), South-East Asia (4.8) and Europe (0.5) . In Africa, leptospirosis has been reported in almost all geographic zones. Despite its high burden, leptospirosis is not routinely diagnosed in African hospitals. Awareness of this disease is also generally lacking among health providers, medical personnel and the general public including high-risk populations such as abattoir workers and animal handlers (Mgode, personal observation). One of the major factors limiting diagnosis of leptospirosis in Africa is the need for leptospire isolation to discover the local circulating serovars that are needed for inclusion in the microscopic agglutination test (MAT). MAT requires various live Leptospira serovars as antigens to detect infections caused by different serovars belonging to different serogroups [3, 4].
Apart from serological studies, there are relatively few studies on isolation and identification of Leptospira pathogens in Africa. However, a number of Leptospira serovars have been isolated in some African countries, namely South Africa [5, 6], Zimbabwe [7, 8], Congo DRC , Kenya [10, 11], Madagascar and other Indian ocean Islands [12, 13], Nigeria and Ghana [9, 14, 15], Egypt  and Tanzania. In Tanzania, leptospirosis is widely reported in wild small mammals, domestic animals and humans [17–22]. Despite these reports, awareness of this disease is still lacking and there is an urgent quest for gathering sufficient data on leptospirosis for promoting awareness. The objectives of this study were, therefore, to determine Leptospira serovars occurring in Tanzania and their host animals. This knowledge will help to rationally design control and prevention measures and contribute to an improved MAT for diagnostic and prevalence study purposes in Tanzania and potentially other East African countries.
Materials and Methods
Domestic and wild animal sampling
Cattle brought at Morogoro municipal abattoir and pigs slaughtered at two main informal slaughterhouse sites also in Morogoro were randomly sampled for this study. Sheep, goats, dogs and cats were also sampled from different localities in Morogoro. Trapping of rodent species and insectivore shrews was stratified whereby rodents were trapped in selected localities representing all geographic areas of Morogoro town including peri-urban areas, urban areas, inside houses, around houses (outdoors), fallow land, swampy areas, inside and around markets, inside and around the abattoir. Sherman live traps baited with peanut butter mixed with maize bran were used to trap small rodents and insectivores (shrew) species. Larger rodents particularly the African giant pouched rats were trapped in same localities as small rodents using Havahart traps baited with fresh maize cobs. The traps were set for three consecutive nights at each site. All captured animals were identified to genus level and geographic coordinates of the collection site were recorded using GPS.
Blood samples for serological determination of leptospirosis by microscopic agglutination test were obtained from patients providing blood in various hospitals in Morogoro for other tests such as diagnosis of typhoid fever. Participants were orally informed that their samples would be anonymously tested for leptospirosis. 3–4 ml of blood was obtained and a drop was inoculated into fresh medium for isolation of leptospires. The remaining blood was centrifuged to obtain serum for serological test. Urine from abattoir workers was collected into sterile universal bottles and transported to the laboratory for inoculation of drops into sterile EMJH medium.
Isolation of leptospires from animals
The isolation of leptospires from animal hosts in Tanzania started in 1996 and is ongoing. Isolation and identification of leptospires have been carried out in humans, domestic animals including cattle and pigs, and feral and (semi) domestic small mammals collected in natural landscapes, agricultural fields, in rural settlements and in urban areas. Wild and domestic animal collection and handling followed the guidelines of the American Society of Mammalogists . Urine specimens were aseptically collected from animals anesthetised using di-ethyl ether. The urine was collected using sterile syringes and needles. Urine sampling was also done from cattle at slaughterhouse whereby the urinary bladder were taken out slaughtered animals and the neck of the bladder was tightly closed with fishing line (thread) to prevent spillage of urine during transportation to the laboratory. A drop of fresh urine was aseptically taken from the bladder using sterile syringe and needle and inoculated into a tube containing sterile Leptospira Ellinghausen and McCullough, modified by Johnson and Harris (EMJH) culture medium containing 5-Fluorouracil selective inhibitor. Kidney specimens were obtained after swabbing the sacrificed animal abdomen with 70% ethanol and dissecting using pair of sterile scissors and forceps. Smaller kidneys were put into sterile glass tube containing sterile phosphate buffered saline (pH 7.0) and homogenised using sterile glass rods and or sterile glass Pasteur pipettes. Larger kidneys were macerated to obtain cross-sectional pieces which were homogenized. A drop of kidney homogenate was aseptically inoculated into EMJH medium as previously described . Cultures were incubated at 30°C for up to 8 weeks and examined weekly for Leptospira growth. Isolation of leptospires from fish species was not conducted in the present study whereas serological testing using putative prevalent serovars indicated potential to provide first insight on leptospirosis in fishes from this area.
Identification of Leptospira isolates
Initially, five Leptospira isolates which were the first isolates from Tanzania of which three were from cattle and two from rodents were identified and enabled identification of many other isolates among the 52 reported in this study. Leptospira isolates SH9 and SH25 from the African giant pouched rats (Cricetomys sp.) and RM1 from cattle were subjected to standard taxonomical analyses recommended by the International Committee on Systematics of Prokaryotes: Subcommittee on the Taxonomy of Leptospiraceae. These were identified as serovar Kenya  and serovar Sokoine . This enabled assigning other serologically and genetically identical isolates among the 52 isolates to serovar Kenya and Sokoine . Isolates coded RM4 and RM7 were subjected to serological typing using serogrouping using reference rabbit serum and monoclonal antibodies. Multilocus sequence typing was also employed to identify sequent isolates from wild rodents and insectivores (Crocidura spp.) from Tanzania through determination of their genetic relatedness with known serovars. This enhanced assigning subsequent isolates to serovars Mwogolo, Lora, Kenya, Qunjian (Canicola) and Sokoine . The typical identification procedures were as follows:
Selected Leptospira isolates coded RM1, RM4 and RM7 from cattle and SH9 and SH25 from the African giant pouched rats (Cricetomys sp.) were grown in EMJH medium for 5–7 days at 30°C. Fully-grown cultures with density of 3x108 leptospires per ml were checked for purity under-darkfield microscopy before injecting into pair of healthy and leptospirosis-free animals to produce antiserum for serological identification of the isolates . Animals were handled in compliance with the “Animal Research: Reporting In Vivo Experiments” (ARRIVE guidelines) and the Helsinki Declaration [27, 28]. The isolates were thereafter reacted with reference rabbit antiserum for common Leptospira serogroups. MAT was performed as previously described . Findings of this prelinanry reaction were useful in selecting reacting serogroups for further identification of new isolates by monoclonal antibodies and cross-agglutination absorption test (CAAT) which uses antiserum produced using unknown (new isolates) and reference serovars as described below.
Serotyping with monoclonal antibodies
MAT sets of specific monoclonal antibodies belonging to candidate Leptospira serogroups were used to determine isolate affiliation. Two isolates coded RM4 and RM7 were subjected to this approach employing the following monoclonal antibodies for serogroup Grippotyphosa: F71C2-4, F71C3-3, F71C9-4, F71C13-4, F71C16-6, F71C17-5, F164C1-1, F165C1-4, F165C2-1, F165C3-4, F165C7-5, F165C8-3 and F165C12-4. Other monoclonal antibodies used were of serovar Butembo serogroup Autumnalis: F43C9-5, F46C1-1, F46C2-4, F46C4-1, F46C5-1, F46C9-1, F46C10-1, F48C1-3, F48C3-3, F48C6-4, F58C1-2, F58C2-3 and F61C7-1. The monoclonal antibodies were provided by the WHO/FAO/OIE Collaborating Centre for Reference and Research on Leptospirosis, at the Royal Tropical Institute, Amsterdam, The Netherlands, which offers varieties of reference leptospirosis research materials worldwide .
Leptospira isolates coded SH9 and SH25 were also subjected to DNA fingerprinting described by Zuerner and Bolin [30, 31] and had identical DNA pattern of serovar Kenya . Isolates coded TE 0826 and TE 0845 have been previously identified using multilocus sequence typing as identical to serovar Mwogolo serogroup Icterohaemorrhagiae; isolates TE 1992, TE 2324, TE 2364 and TE 2366 as serovar Lora serogroup Australis; and isolate coded TE 2980 as serovar Qunjian . Additionally, 3 isolates were previously identified using multilocus sequence typing as serovar Sokoine, and 11 isolates as serovar Kenya .
Cross agglutination absorption test (CAAT)
Further identification of Leptospira isolates was achieved using the gold standard test for identification and taxonomy of Leptospira serovars known as cross agglutination absorption test (CAAT). Briefly, isolates are identified as different serovars if more than 10% of homologous titre remains in one of the test isolates after cross-absorption with sufficient amount of heterologous antigen. This means that 0–10% difference in antibodies remaining following absorption represents strains belonging to same serovar . Leptospira isolate is grown into EMJH medium to density of 3x108 leptospires per ml for inoculation into laboratory rabbits to produce antibodies (antisera) against the isolate. Antiserum is harvested from rabbit and a titre of 1:5120 is determined by MAT using formalin killed homologous isolate. Antiserum with higher titre than 1:5120 is diluted with phosphate buffered saline. The test isolate cultured for 5–7 days in EMJH medium reaching a density of 3x108 leptospires per ml is killed by mixing with formalin (final concentration of 0.5%) and incubating at room temperature for 1 hour. Formalized culture is divided into 5, 10 and 20 ml and centrifuged in refrigerated centrifuge at 10,000 rpm x g for 30 minutes to obtained sediment. The culture sediment is air dried and resuspended into PBS-formalin diluted antiserum. The suspension is incubated at 30°C overnight and thereafter centrifuged at 10,000 rpm x g for 30 minutes to obtain the supernatant which is the now the absorbed serum for MAT checking for absorption levels (under or over absorption) using live and killed antigen similar to the absorbing antigen. The supernatant with titre of 1:40–1:80 that is lower than 1% of homologous titre for the same antiserum will be chosen for control MAT with unabsorbed diluted reference antiserum with live and killed homologous antigen; and MAT with absorbed serum with live and killed homologous reference antigen. Subsequently, the produced antiserum against unknown isolate is absorbed with all positive Leptospira serovars to determine titres remaining after absorption. Detailed procedures of cross-agglutination absorption test have been described by Hartskeerl and co-workers . Leptospira isolates coded SH9 and SH25 from the African giant pouched rats and isolate coded RM1 from cattle in Tanzania were identified as serovar Kenya and serovar Sokoine by this method [18, 19].
Isolates deposit in culture collection
The reference Leptospira serovar Sokoine strain RM1 which is a new serovar described in 2006 has been deposited in Leptospira culture collection at the WHO/FAO/OIE Collaborating Centre for Reference and Research on Leptospirosis of the Royal Tropical Institute, Amsterdam, The Netherlands, and the WHO Collaboration Centre for Diagnosis, Reference, Research and Training in Leptospirosis, Port Blair, Andaman and Nicobar Islands, India . Serovar Kenya strain SH9 and SH25 and as well as serovars Grippotyphosa strain RM4 and RM7, Mwogolo, Lora and Canicola reported in this study have also been deposited in the Leptospira culture collection of the Royal Tropical Institute, Amsterdam, The Netherlands. The isolates are also maintained in the culture collection of the Pest Management Centre, Sokoine University of Agriculture, Morogoro, Tanzania.
Distribution of Leptospira serovars in different wild and domestic mammals, fish and humans
Infection with local Leptospira serogroups and putative serovars in animals and humans was deduced serologically using MAT on blood samples from cattle, rodents, bats, fish and humans. Local Leptospira serovars included in the MAT were Sokoine, Kenya, Lora, Canicola and Grippotyphosa, and reference serovars were Hebdomadis, Pomona and Hardjo.
The Ethical Review Board of Sokoine University of Agriculture approved use of animals. The Tanzania Commission for Science and Technology (COSTECH) granted the research permit for use of wild animals (permit no. 2013-260-NA-2014-110). Infected animals were also handled in compliance with the “Animal Research: Reporting In Vivo Experiments” (ARRIVE guidelines) and the Helsinki Declaration [27, 28]. Wild and domestic animal collecting and handling followed the guidelines of the American Society of Mammalogists . Anonymous human participants gave oral consent allowing anonymous screening for leptospirosis and determination of the prevalence. These individuals were those seeking diagnosis of other diseases in the blood at hospitals and abattoir workers.
Isolation of leptospires from animals
A total of 52 Leptospira isolates were obtained from urine and kidneys of different animal species in Tanzania. The isolation rate of leptospires from different animal hosts ranged from 0.6% in the rodent Mastomys natalensis to 8.4% in the African giant pouched rat (Cricetomys sp.) (Table 1).
Isolation of leptospires from humans
Four Leptospira isolates were obtained from 589 human urine samples that is 0.67% isolation success rate. Eighty-three of the 589 human urine samples were from abattoir workers handling and slaughtering cattle at Morogoro municipal abattoir. Three of the 83 (3.6%) abattoir workers were culture positive. Abattoir workers thus yielded more positive cultures than participants sampled in hospitals (n = 506) from which only one isolate was obtained from an individual living at Kidodi village in the Kilombero river valley that is 150 km away from Morogoro municipality where three isolates were obtained in abattoir workers. The overall isolation rate from both abattoir workers and individuals sampled in hospitals was low (0.19%) with four isolates from 589 individuals. Culturing from fresh 358 blood samples collected in hospitals was negative. The positive cultures from human urine were contaminated and isolates died before carrying out identification.
Common Leptospira serovars with their respective animal hosts were: Sokoine (cattle and rodents); Kenya (rodents and shrews); Mwogolo (rodents); Lora (rodents); Qunjian (Canicola) (rodent); serogroup Grippotyphosa (cattle); and an unknown serogroup or serovar from pigs (Table 2), which is not related to common serogroups or serovars currently reported from Tanzania.
The majority of the 52 Leptospira isolated obtained in this study were from the African giant pouched rat (Cricetomys sp.) which yielded 24 isolates out of 285 specimens (8.42%) and shrews with 11 isolates from 298 specimens (3.7%). Eight isolates were obtained from 1382 Mastomys natalensis rats (0.6%), whereas isolation from 1021 cattle and 236 pigs sampled in cattle slaughterhouse and informal pig slaughterhouses yielded 8 isolates (0.68%) and 2 isolates (0.6%), respectively. Three isolates were obtained from Rattus rattus but cultures were contaminated before performing and preliminary identification hence they are not presented in this work. No isolates were obtained from Lemniscomys spp., Tatera spp., Mus spp. collected in Morogoro municipality. The pattern of Leptospira isolation rates for different animal species is shown in Fig 1.
The preliminary serogrouping of the isolates showed that the RM1 isolate reacts with serum for serogroups Canicola, Icterohaemorrhagiae and Sarmin. The titres for serogroup Icterohaemorrhagiae were higher than those of other serogroups (Table 3). Isolates RM4 and RM7 reacted with rabbit serum for serovar Butembo serogroup Autumnalis as well as with serovar Grippotyphosa and Huanuco of serogroup Grippotyphosa, and to some extent, with serovar Djasiman serogroup Djasiman. Isolates coded SH9 and SH25 reacted with rabbit serum for serovars Kenya and Ballum of serogroup Ballum, and serovar Poi serogroup Javanica (Table 3).
Serotyping with monoclonal antibodies
Leptospira isolates assigned to tentative serogroups in preliminary serogrouping with reference rabbit serum were further analysed using specific monoclonal antibodies for those serogroups. Isolates coded RM4 and RM7 did not react with monoclonal antibodies for serogroup Autumnalis, virtually excluding that they belonged to this serogroup. However, they reacted with 11 of the 13 monoclonal antibodies for Grippotyphosa (Fig 2), supporting that they belong to this serogroup (Table 4). Reaction profiles of RM4 and RM7 were most comparable with that of reference Leptospira serovar Grippotyphosa serogroup Grippotyphosa.
11 of 13 monoclonal antibodies reacted with these isolates.
Distribution and seroprevalence of Leptospira serovars in different wild and domestic mammals, fish and humans
Serological tests involving eight commonly occurring Leptospira serovars (Table 5) in the Morogoro region revealed variations in occurrence and prevalence of Leptospira serovars in wild and domestic mammals, fish and humans. Some Leptospira serovars were found often in more than one animal species whereas other serovars were detected in relatively few animal species. Serovars found in different animal species were serovar Kenya and serovar Sokoine detected in domestic mammals, rodents, bats, fish and humans (Table 5).
The seroprevalence of different Leptospira serovars in different animal species shows varying seropositivity which indicate that these serovars can be used in subsequent MAT for diagnosis of leptospirosis in animal species reported hereunder (Fig 3). An over 10-fold increase in seroprevalence of leptospirosis in humans, wild and domestic mammals in Tanzania was observed following the use of local serovars such as serovar Sokoine in MAT compared to the reference serovar Icterohaemorrhagiae antigen used in the first study of leptospirosis in animals and humans in Tanzania . These observed increases in rodents went from 1.9% to 16.9%, in humans from 0.26% to 10.75% and in dogs from 37% to 39%. There was also an increase in seroprevalence in MAT with the local Grippotyphosa antigen compared to the reference serovar Grippotyphosa as follows: in rodents from 0% to 2%, in dogs from 0% to 10%, and slight increase was observed in humans from 0.26% to 0.5%. Use of the local serovar Kenya in the MAT of goats, sheep, pigs and dogs also yielded higher prevalence (Table 4), which unfortunately lack comparison since the reference serovar Kenya was not tested in Tanzanian animals.
Fifty-three (75.7%) of the 70 seropositive humans and 31 (62%) of the 50 seropositive animals had lower antibody levels (1:20–1:80) against eight tested Leptospira serovars. These titres are below the cut-off point of 1:160 adopted from European setting which has been in use in Tanzania for past two decades due to absence of intensive leptospirosis studies determining cut-off point for Africa. Serovar Sokoine was the most reacting serovar in both humans and animals and contributed to 62.3% (33 out of 53) and 38.7% (12 out of 31) of the seropositivity with lower titres. Majority of the higher titres in 10 out of 17 humans (58.8%) and 13 out of 19 (68.4%) rodents was due to serovar Sokoine. This was followed by serovar Hardjo that contributed to 15% of lower titres and 23.5% (4 out of 17) of the higher titres in humans. Serovar Qunjian (Canicola) contributed to 29% (9 out of 31) lower titres and 21% (4 out of 19) of the higher titres in rodents. Serovar Grippotyphosa also contributed to 29% (9 out 31) lower titres in rodents and 5% (1 out of 19) of the higher titres in these animals.
Leptospira serovars for use in MAT in African region
The following Leptospira serovars (Table 6) belonging to different species and serogroups yields high positivity when used in MAT of humans and broad range of animal species. Although not exhaustive the listed representative serovars cross reacts with at least 10 other serovars previously reported in central and eastern Africa, Indian ocean islands located near eastern Africa coast, and elsewhere. For example, serovar Sokoine that is widespread in various domestic and wild animal species in Tanzania (Table 5) reacts with serovars Mwogolo, Ndahambukuje and Ndambari found in Congo DRC in central Africa , and reacts also with serovars Copenhageni and Icterohaemorrhagiae all belonging to serogroup Icterohaemorrhagiae. Serovar Sokoine again reacts with serovars Weaveri and Rio of serogroup Sarmin as demonstrated in MAT for preliminary serogrouping (Table 3). This cross reactivity broadens detection of leptospirosis caused by these serovars in MAT using serovar Sokoine. Serovar Kenya widely found in rodents in Tanzania was first described in neighbouring Kenya . Its wide distribution in eastern Africa region makes it a good candidate for inclusion in MAT in this region. Serovar Grippotyphosa isolated in cattle in Tanzania cross-reacts with serovar Butembo found in Congo DRC in central Africa which widens the geographic region that this serovar can be applied in MAT. Isolation of additional serovars from Africa is much needed to establish a comprehensive region-specific Leptospira serovars for successful leptospirosis diagnosis in African region.
The proportion of prevalence of the Leptospira serovars recommended for diagnosis of leptospirosis in humans and different animal species is indicated in Fig 3. Leptospira serovar Pomona was absent in African giant rats, shrews (Crocidura spp.) and bats. Serovar Hebdomadis was not detected in bats and fish whereas Canicola was negative in shrews (Crocidura spp.) and bats. Serovar Hardjo was negative in rodent species and Grippotyphosa was not detected in shrew species. Leptospira serovars, which did no react with tested animal species, are not presented in Fig 3 below.
This study shows that diverse Leptospira serovars occur in a wide range of wild and domestic mammal species, fish and humans in Tanzania. The local Leptospira serovar Sokoine and serovar Kenya were the predominant serovars found in many vertebrate species, including fish and humans. Serovar Sokoine for example has been isolated from cattle, rodents (Mastomys natalensis and Cricetomys sp.) and shrews (Crocidura sp.). This serovar has also been detected serologically in humans, cattle, rodents, shrews, bats and fish [20, 21]. The distribution pattern of Leptospira in different animals species determined by their isolation rate and seroprevalence indicates that certain rodent species harbour leptospires more often than other species. For example, Mastomys natalensis, which are the most abundant rodent species in sub-Saharan Africa  yielded few Leptospira isolates and had low seroprevalence compared to the African giant pouched rat (Cricetomys sp.) and shrews (Crocidura sp.), which are also widely distributed across Africa. This lower infection rate in Mastomys natalensis could be due to differences in habitats where these species are found, differences in foraging behaviours and/or physiology. For example, Cricetomys sp. lives in burrows, which in urban areas may extend to pit latrines and garbage collection areas where they forage. These habitats potentially increase the chances of contracting leptospires and may explain the high isolation rates observed in Cricetomys sp. and Crocidura sp. (Fig 1). Similarly, Crocidura species often appear to live in moist areas. Shrews feed on insects found on soils and wet or moist environments which is reported to support the survival of leptospires for relatively longer periods of time [37, 38]. On the other hand, Mastomys natalensis habitats are relatively different from those of Cricetomys sp. and Crocidura sp. and is considered a peridomestic rodent found in both wild habitats such as shrubs and grasslands as well as crop fields and houses . This study indicates that Cricetomys sp. and Crocidura sp. serve as major reservoirs of leptospirosis among small mammal species. Future studies aiming at isolation of leptospires to determine serovar prevalence in neglected regions should target the giant African pouched rats (Cricetomys sp.) and shrew species (Crocidura sp.) or other animal species with similar life styles, e.g. Rattus norvegicus.
This study shows that certain Leptospira serovars are specific to certain animal species but that some serovars such as Sokoine and Kenya are found in a broad range of animal species including domestic animals, rodents, bats and fish. Leptospira isolates belonging to serovars Sokoine and Kenya were serologically detected by MAT in diverse animal species including cattle, sheep, goats, dogs, cats, rodents, bats, fish and humans (Table 5), (Fig 3). Serovar Sokoine belongs to serogroup Icterohaemorrhagiae that majority of its serovars are often reported in humans worldwide . Furthermore, serovars Sokoine and Kenya belong to the L. kirschneri species that is considered predominant in the East and Central African region including Indian Ocean islands near the East African coast [9, 13]. Other Leptospira serovars encountered in animals and humans include serovars Hebdomadis, Hardjo, Pomona, Lora, Australis and Canicola. The seroprevalence of these serovars in different animal species and humans shows relatively lower prevalence compared to the proportions of serovar Sokoine, Kenya and Lora. The observed occurrence and prevalence of these serovars in animals and humans indicate that they are major candidate serovars for inclusion and use as antigens in subsequent MAT for serodiagnosis of leptospirosis in animals and humans in this region. Studies focusing in isolation of new Leptospira serovars in humans and animals in Africa are urgently needed to generate a panel of region-specific Leptospira serovars for MAT in African continent. In this study inclusion of local serovars, particularly serovar Sokoine, in MAT detection of leptospiral antibodies in rodents and humans in Tanzania revealed an over 10-fold increase in leptospirosis prevalence which was higher than the prevalence reported in the first broad study of leptospirosis in Tanzania . An increase in seroprevalence was also observed following use of the local serovar Grippotyphosa in determination of leptospirosis in humans and animals. Similarly, the local serovar Kenya also demonstrated higher leptospirosis prevalence in goats, sheep, pigs and dogs exceeding those of reference serovars Hebdomadis, Pomona, Hardjo and Canicola (Table 5). This further indicates the necessity for isolation of local Leptospira for use in MAT.
Majority of seropositive humans and animals particularly rodents had lower titres against the tested serovars whereas serovar Sokoine and Hardjo had the highest number of individuals with lower and higher titres in humans. Serovar Sokoine had also the highest number of animals with lower and higher titres followed by serovar Canicola. Serovar Grippotyphosa had also higher number of animals with lower titres. Serovar Hardjo was not detected in rodents. These findings indicate the need for establishing the cut-off point for serological diagnosis (MAT) of leptospirosis in humans and animals in Africa where the disease in endemic due to abundance and diversity of reservoir hosts in Africa. Emphasize is needed to isolate and determine antibody levels using animals’ seropositivity and titres, which are common in animals yielding positive isolates.
The findings suggest potential risk of human infection from animal leptospirosis indicated by isolation of three Leptospira isolates from urine of three abattoir workers out of 83 individuals (3.6%) sampled among people involved with slaughtering of cattle at Morogoro abattoir where 12 Leptospira isolates belonging to serovar Sokoine, Grippotyphosa and Qunjian (Canicola) were isolated from cattle and rodents captured around the abattoir. Leptospira isolation success of 3.6% in abattoir workers indicates higher infection risk in this population than in the general population in which only one sample was culture positive (0.19%) out of 506 urine samples collected from patients taking blood tests in hospitals. Indeed the overall rate of Leptospira isolation from abattoir workers and other participants from hospitals was lower (0.67%) compared to 3.6% positivity observed in abattoir workers. Abattoir workers rarely ware adequate personal protective gears that can prevent direct contact with animals’ blood and urines when working at this abattoir and other two informal pig slaughterhouses where leptospires were isolated from pigs also in Morogoro. Successful isolation of leptospires from rodents captured inside and around houses which increases the risk of human infections. The observed lower antibody levels in humans may also indicate consistent exposure to leptospires. Isolation of leptospires from a patient at Kidodi village located 150 km away from Morogoro town further indicates high risk of leptospirosis although the identification of the four human isolates was not successful as they died from contamination before preliminary identification. Kidodi village is located along the Kilombero valley where sugarcane farming is the main agricultural activity that is associated with Leptospira infection.
Two Leptospira isolates obtained from pigs appear to differ from serovars belonging to serogroups Grippotyphosa, Icterohaemorrhagiae and Ballum. The two isolates from pigs did not react with any of the reference rabbit serum for serovars belonging to these serogroups including serum against the most common Leptospira serovars Sokoine and Kenya. Further identification of these isolates is required to understand their taxonomic status for serodiagnostic and epidemiological purposes. Furthermore, there is an urgent need for conducting leptospirosis studies focusing on isolation and identification of leptospires from a wide range of terrestrial and aquatic animal species in understudied areas of the African continent. Such studies may enhance mapping of the distribution pattern of Leptospira serovars and the actual burden of this disease across Africa. This could be achieved by establishing Leptospira isolation facilities in microbiological laboratories, especially in universities and research institutions existing in different African countries. Successful isolation should be followed by preliminary identification of the isolates to at least genus level using darkfield microscopy. Subsequently, the isolates could be identified to serogroup level by MAT as shown in this report (Table 3). The new isolates should also be inoculated into rabbits to produce anti-leptospira antibodies for use in serological typing and MAT . These experimental steps are feasible in most African countries. Further identification of isolates could also be achieved using molecular DNA fingerprinting methods [30, 31] which can enhance comparisons of DNA fingerprint patterns of known serovars with unknown isolates from similar localities prior to the gold standard cross agglutination absorption test (CAAT) recommended for taxonomy of the leptospires .
In conclusion, diverse Leptospira serovars occur in animals and humans in Tanzania. These Leptospira serovars have implications in serodiagnosis of this zoonotic disease in both animals and humans. Serovars Sokoine, Kenya, Grippotyphosa, Lora, Pomona, Hardjo, Hebdomadis and Canicola should be included in leptospirosis diagnosis in Tanzania and neighbouring countries. Further studies focusing on isolation and identification of leptospires from terrestrial and aquatic animal species as well as humans are needed to understand potential circulating serovars in neglected regions where the disease is not recognised and not routinely diagnosed in hospitals. A recent study of causes of fevers among infants and children in northern Tanzania shows that 7.7% were due to leptospirosis . This prevalence could increase when local Leptospira serovar Sokoine is used as antigen as has been demonstrated in humans from Morogoro region where initial surveillance conducted in 1996 using reference serovars showed lower prevalence (0.26%) , and subsequence surveillance conducted in 2006 using local serovar Sokoine showed higher prevalence (10.7%) . Similar trend was recently observed in rodents whereby previous studies using reference serovar Icterohaemorrhagiae belonging to serogroup Icterohaemorrhagie of which serovar Sokoine also belongs was 5%  and a higher prevalence (16.9%) was obtained when local Leptospira serovar Sokoine was used in rodent population located 30 km away from where serovar Sokoine was isolated in Morogoro, Tanzania . Generally, this study shows that use of local serovar Sokoine and Kenya in MAT reveals high leptospirosis prevalence in wide range of animal species and calls for reconsideration of previous knowledge that certain Leptospira serovars infects only certain animal species. Serovar Sokoine in this case was found in humans, domestic animals (including pet animals), rodents, bats and fishes, hence making it a broad antigen for leptospirosis diagnosis in Africa.
Public awareness of leptospirosis should be promoted to high-risk populations including farmers, livestock keepers, fishermen and abattoir workers. Leptospirosis has been reported also in residents of rural and urban areas interacting with rodents but not engaged with risk occupational activities . Hospital staff, clinicians, veterinarians and policy makers’ needs awareness of existence and high prevalence of leptospirosis in Africa and should consider its diagnosis and treatment. For example in Tanzania and neighbouring countries, diagnosis of leptospirosis in hospitals can be achieved in collaboration with the leptospirosis laboratory at Sokoine University of Agriculture. Capacity building training on leptospirosis diagnosis, Leptospira isolation and maintenance of Leptospira cultures for use as live antigens for leptospirosis diagnosis should be emphasized in Africa in order to successful control this debilitating and fatal neglected disease.
S1 Flowchart. Flowchart of leptospirosis study in humans.
S2 Flowchart. Flowchart of leptospirosis study in rodents and shrews.
Authors wish to thank the staff of the Royal Tropical Institute (KIT)-Biomedical Research Department (The Netherlands) and Sokoine University of Agriculture, Pest Management Centre for their cooperation.
Conceived and designed the experiments: GFM RSM HL RAH SRB. Performed the experiments: GFM GGM AK LD. Analyzed the data: GFM LSM SRB. Contributed reagents/materials/analysis tools: RAH LSM RSM. Wrote the paper: GFM SRB RAH RSM HL.
- 1. Pappas G., Papadimitriou P., Siozopoulou V., Christou L. & Akritidis N. (2008) The globalization of leptospirosis: worldwide incidence trends. International Journal of Infectious Diseases 12, 351–357. pmid:18055245
- 2. World Health Organization. (2011) Report of the second meeting of leptospirosis burden epidemiology reference group. Geneva, Switzerland: World Health Organization.
- 3. Cole J.R., Sulzer C.R. & Pursell A.R. (1973) Improved microtechnique for the leptospiral agglutination test. Applied Microbiology 25, 976–980.
- 4. Goris M.G. & Hartskeerl R.A. (2013). Leptospirosis serodiagnosis by the microscopic agglutination test. Current Protocols in Microbiology 12E–5.
- 5. Herr S, Riley AE, Neser JA (1982). Leptospira interrogans serovar pomona associated with abortion in cattle: isolation methods and laboratory animal histopathology. The Onderstepoort Journal of Veterinary Research 49(1): 57–62. pmid:7122066
- 6. Brugge LA, Dreyer T (1985). Leptospira interrogans serovar hardjo associated with bovine abortion in South Africa.The Onderstepoort Journal of Veterinary Research 52(1): 51–52. pmid:4011157
- 7. Feresu S.B., Bolin C.A. & Korver H. (1995). Identification of leptospires of the Pomona and Grippotyphosa serogroups isolated from cattle in Zimbabwe. Research in Veterinary Science 59: 92–94. pmid:8525094
- 8. Feresu S. B., Bolin C. A., & Korver H. (1998). A new leptospiral serovar, ngavi, in the Tarassovi serogroup isolated from Zimbabwe oxen. International journal of systematic bacteriology, 48(1), 207–213.
- 9. Faine S., Adler B., Bolin C. & Perolat P. (1999) Leptospira and Leptospirosis. Melbourne: MediSci.
- 10. Kranendork O., Wolff J.W., Bohlander J.W., Roberts J.M.D., De Geus A. & Njenga R. (1968) Isolation of new Leptospira serovars in Kenya. World Health Organization (WHO) Zoonotics 111, 1–5.
- 11. Dikken H, Timmer VE, Njenga R (1981). Three new leptospiral serovars from Kenya. Tropical and Geographical Medicine 33(4):343–346. pmid:7342381
- 12. Rahelinirina S, Léon A, Harstskeerl RA, Sertour N, Ahmed A, et al., (2010) First isolation and direct evidence for the existence of large small-mammal reservoirs of Leptospira sp. in Madagascar. PLoS ONE 5(11): e14111. pmid:21124843
- 13. Bourhy P., Collet L., Clement S., Huerre M., Ave P., Giry C., Pettinelli F. & Picardeau M. (2010) Isolation and characterization of new Leptospira genotypes from patients in Mayotte (Indian Ocean). PloS Neglected Tropical Diseases 4, e724. pmid:20582311
- 14. Hogerzeil H.V., De Geus A., Terpstra W.J., Korver H., Ligthart G.S. (1986) Leptospirosis in rural Ghana: Part 2, Current leptospirosis. Tropical and Geographical Medicine 38(4):408–414. pmid:3810845
- 15. Ezeh AO, Adesiyun AA, Addo PB, Ellis WA, Makinde AA, Bello CS (1991). Serological and cultural examination for human leptospirosis in Plateau State, Nigeria. The Central African Journal of Medicine 37(1):11–15. pmid:2060002
- 16. Felt S.A., Wasfy M.O., El-Tras W.F., Samir A., Rahaman B.A., Boshra M., Parker T.M., Hatem M.E., El-Bassiouny A.A., Murray C.K. & Pimentel G. (2011). Cross-species surveillance of Leptospira in domestic and peri-domestic animals in Mahalla City, Gharbeya Governorate, Egypt. American Journal of Tropical Medicine and Hygiene 84 (3): 420. pmid:21363980
- 17. Machang’u R.S., Mgode G. & Mpanduji D. (1997) Leptospirosis in animals and humans in selected areas of Tanzania. Belgian Journal of Zoology 127, 97–104.
- 18. Machang'u R.S., Mgode G.F., Assenga J., Mhamphi G., Weetjens B., Cox C., Verhagen R., Sondij S., Goris M.G. & Hartskeerl R.A. (2004) Serological and molecular characterization of Leptospira serovar Kenya from captive African giant pouched rats (Cricetomys gambianus) from Morogoro Tanzania. FEMS Immunology and Medical Microbiology 41, 117–121. pmid:15145455
- 19. Mgode G.F., Machang’u R.S., Goris M.G., Engelbert M., Sondij S. & Hartskeerl R.A. (2006) New Leptospira serovar Sokoine of serogroup Icterohaemorrhagiae from cattle in Tanzania. International Journal of Systematic and Evolutionary Microbiology 56, 593–597. pmid:16514033
- 20. Mgode G.F., Mbugi H.A., Mhamphi G.G., Ndanga D. & Nkwama E.L. (2014). Seroprevalence of Leptospira infection in bats roosting in human settlements in Morogoro municipality in Tanzania. Tanzania Journal of Health Research 16 (1).
- 21. Mgode G. F., Mhamphi G. G., Katakweba A., & Thomas M. (2014b). Leptospira infections in freshwater fish in Morogoro Tanzania: a hidden public health threat. Tanzania Journal of Health Research, 16(2).
- 22. Biggs H.M., Bui D.M., Galloway R.L., Stoddard R.A., Shadomy S.V., Morrissey A.B., Bartlett J.A., Onyango J.J., Maro V.P., Kinabo G.D., Saganda W. & Crump J.A. (2011) Leptospirosis among hospitalized febrile patients in northern Tanzania. American Journal of Tropical Medicine and Hygiene 85, 275. pmid:21813847
- 23. Gannon W. L., & Sikes R. S. (2007). Guidelines of the American Society of Mammalogists for the use of wild mammals in research. Journal of Mammalogy, 88(3), 809–823.
- 24. Mgode G.F., Mhamphi G., Katakweba A., Paemelaere E., Willekens N., Leirs H., Machang’u R.S. & Hartskeerl R.A. (2005) PCR detection of Leptospira DNA in rodents and insectivores from Tanzania. Belgian Journal of Zoology 135, 17–19.
- 25. Ahmed N., Devi S.M., Valverde Mde L., Vijayachari P., Machang'u R.S., Ellis W.A. & Hartskeerl R.A. (2006) Multilocus sequence typing method for identification and genotypic classification of pathogenic Leptospira species. Annals of Clinical Microbiology and Antimicrobials 5, 28. pmid:17121682
- 26. Faine S. (Ed.) (1982) Guidelines for the Control of Leptospirosis. World Health Organization, Geneva.
- 27. World Medical Association (WMA). (2001) World Medical Association Declaration of Helsinki. Ethical principles for medical research involving human subjects. Bulletin of the World Health Organization, 79(4), 373. pmid:11357217
- 28. McGrath J. C., Drummond G. B., McLachlan E. M., Kilkenny C., & Wainwright C. L. (2010) Guidelines for reporting experiments involving animals: the ARRIVE guidelines. British journal of pharmacology, 160(7), 1573–1576. pmid:20649560
- 29. KIT Biomedical Centre, Leptospirosis Reference Centre: Typing with monoclonal antibodies. http://www.kit.nl/biomedical-research/leptospirosis-reference-centre. Visited 30/8/2015.
- 30. Zuerner R.L, Bolin C.A (1995) IS1533-based PCR assay for identification of Leptospira interrogans“sensu lato” serovars. J. Clin. Microbiol. 33, 3284–3289. pmid:8586718
- 31. Zuerner R.L, Bolin C.A (1997) Differentiation of Leptospira interrogans isolates by IS1500 hybridization and PCR assays. J. Clin. Microbiol. 35, 2612–2617. pmid:9316917
- 32. Hartskeerl R. A., Smits H. L., Korver H., Goris M. G. A., Terpstra W. J., & Fernández C. (2001). International course on laboratory methods for the diagnosis of leptospirosis. Netherlands: Royal Tropical Institute Department of Biomedical Research
- 33. Machang’u R., Mgode G., Asenga J., Mhamphi G., Hartskeerl R., Goris M., Cox C., Weetjens B. & Verhagen R. (2003). Characterization of Leptospira isolates from captive giant pouched rats, Cricetomys gambianus. In: Rats, Mice and People, Rodent Biology and Management. (Eds) Singleton GR, Hinds LA, Krebs CJ, and Spratt MD. Australian Centre for International Agricultural Research, Canberra, 2003, pp 40–42. http://projects.nri.org/ecorat/docs/MN96Chapter1.pdf#page=39. Visited 21 June 2014.
- 34. Kessy M. J., Machang’u R. S., & Swai E. S. (2010) A microbiological and serological study of leptospirosis among pigs in the Morogoro municipality, Tanzania. Tropical Animal Health and Production, 42(3), 523–530. pmid:19763865
- 35. Machang’u, R. (2006) Rodent and human disease in Tanzania. RatZooMan Workshop 3–6 May 2006, Malelane, Republic of South Africa, pp 26–27. http://projects.nri.org/ratzooman/docs/workshop_proceedings.pdf. Visited 7 June 2014.
- 36. Christensen J. T. (1996). Home range and abundance of Mastomys natalensis (Smith, 1834) in habitats affected by cultivation. African Journal of Ecology, 34(3), 298–311.
- 37. Smith D. J. W., and Self H. R. M. (1955) Observations on the survival of Leptospira australis A in soil and water. Journal of Hygiene 53 (4): 436–444. pmid:13278528
- 38. Trueba G., Zapata S., Madrid K., Cullen P., & Haake D. (2004). Cell aggregation: a mechanism of pathogenic Leptospira to survive in fresh water. International Microbiology, 7(1), 35–39. pmid:15179605
- 39. Leirs H., Verheyen W., & Verhagen R. (1996). Spatial patterns in Mastomys natalensis in Tanzania (Rodentia, Muridae). Mammalia, 60 (4), 545–556.
- 40. International Committee on Systematics of Prokaryotes: Subcommittee on the Taxonomy of Leptospiraceae. (2008). Intern J of Systematic and Evolutionary Microbiol. 58, 1049–1050.
- 41. Crump JA, Morrissey AB, Nicholson WL, Massung RF, Stoddard RA, et al. (2013) Etiology of Severe Non-malaria Febrile Illness in Northern Tanzania: A Prospective Cohort Study. PLoS Negl Trop Dis 7(7): e2324. pmid:23875053
- 42. Mgode GF, Katakweba AS, Mhamphi GG, Fwalo F, Bahari M et al. (2014). Prevalence of leptospirosis and toxoplasmosis: A study of rodents and shrews in cultivated and fallow land, Morogoro rural district, Tanzania. Tanzania Journal of Health Research, 16(3).
- 43. Vinetz JM, Glass GE, Flexner CE, Mueller P, Kaslow DC (1996). Sporadic urban leptospirosis. Annals of internal medicine, 125(10), 794–798. pmid:8928985