- Research article
- Open Access
Survey of domestic cattle for anti-Leishmania antibodies and LeishmaniaDNA in a visceral leishmaniasis endemic area of Bangladesh
https://doi.org/10.1186/1746-6148-7-27
© Alam et al; licensee BioMed Central Ltd. 2011
- Received: 8 December 2010
- Accepted: 8 June 2011
- Published: 8 June 2011
Abstract
Background
Visceral leishmaniasis (VL), caused by an intracellular parasite Leishmania donovani in the Indian subcontinent, is considered to be anthroponotic. The role of domestic animals in its transmission is still unclear. Although cattle are the preferred blood host for Phlebotomus argentipes, the sandfly vector of VL in the Indian subcontinent, very little information is available for their role in the disease transmission. In this study, we examined domestic cattle for serological and molecular evidence of Leishmania infection in a VL-endemic area in Bangladesh. Blood samples from 138 domestic cattle were collected from houses with active or recently-treated VL and post-kala-azar dermal leishmaniasis patients. The presence of anti-leishmanial antibodies in serum was investigated using enzyme-linked immunosorbent assay (ELISA) and then with direct agglutination tests (DAT). Nested PCR (Ln PCR) was performed to amplify the ssu-rRNA gene using the DNA extracted from Buffy coat. Recently-developed molecular assay loop-mediated isothermal amplification (LAMP) was also performed for further sensitive detection of parasite DNA.
Results
In this study, 9.4% (n = 13) of the cattle were found to be positive by ELISA. Of the 13 ELISA-positive cattle, only four (30.8%) were positive in DAT. Parasite DNA was not detected in either of the molecular assays (Ln PCR and LAMP).
Conclusions
The study confirmed the presence of antibodies against Leishmania parasite in cattle. However, the absence of Leishmania DNA in the cattle indicates clearly that the cattle do not play a role as reservoir host. Similar study needs to be undertaken in the Indian subcontinent to determine the role of other domestic animals on which sandflies feed.
Keywords
- Visceral Leishmaniasis
- Indian Subcontinent
- Cutaneous Leishmaniasis
- Myiasis
- Domestic Cattle
Background
Eighty-eight countries of the world are endemic with either of the two major forms of leishmaniasis: cutaneous leishmaniasis (CL), a disfiguring and stigmatizing disease, and visceral leishmaniasis (VL) or kala-azar, which is fatal if remains untreated [1]. One hundred fifty million people are living with the risk of VL in the Indian subcontinent (India, Nepal, and Bangladesh) [2]. VL leads to a loss of about 400,000 disability-adjusted life-years (DALYs) every year in this region [3]. VL is believed to be anthroponotic in the subcontinent. Results of several studies have shown that Phlebotomus argentipes, the only known vector for Leishmania donovani in the Indian subcontinent, prefer to feed on both bovine and human blood [4–8]. Being a preferable host for P. argentipes, cattle was shown to play an undecided role in several epidemiological studies in the Indian subcontinent [9]. For example, Ownership of cattle in Nepal and its density in Bangladesh were found to be protective [10, 11]. Whereas, increased risk of VL was found to be associated with the density of cattle or its ownership in India [12, 13]. Serological evidences of anti-L. donovani antibodies in different domestic animals including cattle were reported in Sudan [14]. In a recent study in Nepal, Leishmania DNA was detected in several domestic animals including cattle from an endemic area [15]. However, to date, no study has been conducted in Bangladesh to investigate the role of any domestic animal in VL transmission.
This study was aimed to investigate the evidence of anti-leishmanial antibodies in blood of domestic cattle from VL-endemic villages of Mymensingh district in Bangladesh. Molecular diagnostic tests were also performed to detect circulating parasite DNA in blood through polymerase chain reaction (PCR) and loop-mediated isothermal amplification (LAMP).
Methods
Study area
The study was conducted in Trishal upazila (subdistrict) of Mymensingh district in Bangladesh. Trishal has a land area of 339 sq km, with a population of 3.7 million. The annual incidence of kala-azar in Trishal ranges from 21 to 26 per 10,000 people per year [16].
Sample-size
Results of a previous study with domestic and wild animals in Sudan showed that 21.4% had seropositivity against anti-L. donovani antibodies in cows [14]. However, in the absence of a similar study in the Indian subcontinent, we assumed that cattle might show 10% of seropositivity in our study. Based on this assumption, we calculated that 138 cattle would be required for our study [precession 5% and 95% confidence interval (CI)]. Sample-size was calculated using Windows® version of the Epi Info 3.2.2 software.
Sample collection from cattle
Blood samples were collected from cattle during August-September 2008. At the beginning, past (within last 3 months) and active (treatment ongoing or awaiting for treatment) VL and post-kala-azar dermal leishmaniasis (PKDL) patients were identified from the records of Trishal Upazila Health Complex, Mymensingh. A research team, consisting of an experienced veterinary doctor or a veterinary assistant, visited the study houses, enumerated domestic cattle (Bos indicus), and collected five mL of blood from the jugular vein from randomly-selected one from each study house. After collection, three mL of blood was transferred to an EDTA containing tube for Buffy coat separation, and the remaining two mL was transferred to a sterile test tube for serum separation. Relevant information on age, sex, body condition score, etc. and any changes in behaviour within the past six months of the selected cattle were recorded. Their physical condition was scored in the scale of 1-5 (with 0.5 fractions between 2 scores) which represent worst to best physical condition on the basis of bony prominence and deposition of subcutaneous fat [17]. The blood samples were transported to the nearby field office for Buffy coat and serum separation. The processed samples were then preserved at -20°C before transferring these to the Parasitology Laboratory of ICDDR, B in Dhaka for further serological and molecular investigations.
Ethical consideration
The study was approved by the Research Review Committee and the Animal Experimentation Ethics Committee of ICDDR, B. Consent was obtained from the owners of the cattle before the collection of blood sample.
Laboratory investigation
Enzyme-linked immunosorbent assay
For the qualitative detection of antibodies (IgG, IgM, and IgA) against L. donovani in the serum samples, the RecombiLISA Leishmania Ab Test (CTK Biotech Inc., San Siego, USA) was performed. The RecombiLISA Leishmania Ab Test comprises two key components: (a) solid microwells pre-coated with recombinant L. donovani antigens and (b) liquid conjugates composed of recombinant L. donovani antigens conjugated with horse reddish peroxidase (HRP-Leish Ag conjugates). The test was performed by incubating serum and HRP-Leish Ag conjugate in wells of the plate. Antibodies (IgG, IgM, or IgA) to L. donovani in the specimens would react to the L. donovani antigens coated onto the plate well by making complex with the HRP-Leish Ag conjugates. Unbounded conjugates were then removed by washing. After adding substrate and stop solution, the change in color to yellow indicates Ab-positive, and then the absorbance was measured by spectrophotometer at 450 nm absorbance. Duplicate wells were run for each sample.
Interpretation of ELISA results
The ELISA results were interpreted according to the instructions of the manufacturer. Briefly, a cut-off value was obtained from the mean optical density (OD) value of the negative controls + 0.1. Then an OD ratio was calculated for each sample by dividing the mean OD value by the cut-off value. Sample with OD ratio of ≥ 1.00 was considered to be positive, and the OD ratio of < 1.00 was considered to be negative. Serum samples collected from four cattle from a non-endemic area were used as negative controls in each test. Repeated tests were performed with serum samples with a positive result along with an equal number of randomly-selected negative serum samples and negative controls to make a precise conclusion. However, no discrepancy was found in the repeat tests.
Direct agglutination test
The DAT was performed with the serum samples which were found to be positive in the ELISA test, along with a similar number of ELISA-negative samples. Commercially-available DAT antigen (Koninklijk Instituut voor de Tropen, Amsterdam, the Netherlands) was used following the protocol described by Harith et al. [18]. Duplicate wells were run for each of the serum dilution. Heat-inactive fetal bovine serum was used along with physiologic saline and DAT antigen as negative control [19]. An agglutination titer of 1:3200 was considered positive in this study [14].
PCR
DNA from Buffy coat was extracted using QIAamp® DNA blood mini kit (QIAGEN, Düsseldorf, Germany). Nested PCR (Ln PCR) was performed to amplify the ssu-rRNA gene with some modifications of the protocol previously described by Cruz et al. [20]. The first PCR was specific for the order Kinetoplastida using the primer R221 and R332 with a product size of 603 base pair. The second PCR was specific for Leishmania genus using the diluted (1:50) first PCR product using the primers R223 and R333, with the product size of 358 base pair. Briefly, in the first reaction, 2 μL of the extracted DNA, 15 pmol of primers (Kinetoplastida-specific) R221 and R332 were used in 25 μL PCR mix containing 0.2 mM dNTP, 2 mM MgCl2, 5 mM KCl, 75 mM Tris-HCl (PH 9.0), 0.001% bovine serum albumin, 2.0 mM (NH4)2SO4 and 2.5 U of Taq polymerase. For the second reaction, 1 μL of a 1/50 dilution of the first PCR product was used as a template in the presence of 15 pmol of primer R223 and 15 pmol of primer R333 which are Leishmania genus-specific. Reaction conditions are the same as the first PCR. Amplification products were visualized on 1.5% agarose gel using a 100 bp DNA ladder after staining with ethidium bromide (0.1 mg/mL). DNA from in-house-cultured L. donovani was used as a positive control in the PCR assay.
Loop-mediated isothermal amplification
LAMP was performed followed the protocol described by Takagi et al. [21]. In brief, the LAMP reaction was performed in 25 μL of reaction mixture containing 40 pmol each of FIP and BIP primers, 5 pmol each of F3 and B3c primers, 1.4 mM each of deoxynucleoside triphosphate, 0.8 M betaine, 20 mM Tris-HCl, pH 8.8, 10 mM KCl, 10 mM (NH 4)2 SO4, 8 mM MgSO4, 0.1% TritonX-100, 8 units of Bst DNA polymerase large fragment (New England Biolabs, Ipswich, MA), and 2 μL of sample DNA. The mixture was incubated at 65°C for 50 minutes in a heat block. After incubation, the turbidity was examined visually.
Data analysis
Data were computed in the Microsoft Excel software. Frequencies and the association between different variables (chi-square test with Yate's correction and Fisher's exact test) were analyzed using the SPSS software (version 11.5). A p value of < 0.05 was considered significant.
Results
Some characteristics of the study cattle along with ELISA results
Category | Frequency (%) | Positive (%) | ||
|---|---|---|---|---|
Sex | ||||
Male | 50 (36.2) | 5 (3.6) | ||
Female | 88 (63.8) | 8 (5.8) | ||
Age-group (months) | ||||
10 or less | 4 (2.9) | 0 (0) | ||
11-20 | 42 (30.4) | 5 (3.6) | ||
21-30 | 40 (29.0) | 1 (0.7) | ||
31-40 | 23 (16.7) | 1 (0.7) | ||
41-50 | 11 (8.0) | 2 (1.4) | ||
51 plus | 18 (13.0) | 4 (2.9) | ||
Physical condition score | ||||
1 | 17 (12.3) | 0 (0) | ||
2 | 53 (38.4) | 4 (2.9) | ||
3 | 38 (27.5) | 4 (2.9) | ||
4 | 23(16.7) | 4 (2.9) | ||
5 | 7 (5.1) | 1 (0.7) | ||
Lesions | ||||
None | 132 (95.7) | 12 (8.7) | ||
Scar marks | 3 (2.2) | 0 (0) | ||
Myiasis | 2 (1.4) | 0 (0) | ||
Skin rash | 1 (0.7) | 0 (0) | ||
Total | 138 (100) | 13 (9.4) | ||
ELISA reading for the presence of anti L. donovani antibodies
Profile of ELISA-positive cattle
ID | Age (months) | Sex | Colour | PCS* | Variety | Lesion | DAT** titer | DAT result |
|---|---|---|---|---|---|---|---|---|
12 | 36 | Female | Reddish | 2 | Native | Myiasis | 1:1600 | -ve |
17 | 60 | Female | Reddish | 4 | Native | No | 1:800 | -ve |
19 | 72 | Female | White | 5 | Native | No | 1:3200 | +ve |
23 | 12 | Female | White | 3 | Native | No | 1:1600 | -ve |
39 | 18 | Male | Reddish | 3 | Native | No | 1:6400 | +ve |
40 | 18 | Male | Brown | 2 | Red Shindhi | No | 1:1600 | -ve |
44 | 15 | Male | Reddish brown | 2 | Red Shindhi | No | 1:200 | -ve |
45 | 14 | Male | White | 3 | Native | No | 1:3200 | +ve |
85 | 48 | Female | Reddish | 4 | Native | No | 1:1600 | -ve |
89 | 60 | Female | Reddish and white | 3 | Native | No | 1:400 | -ve |
97 | 30 | Male | White | 2 | Native | No | 1:3200 | +ve |
120 | 42 | Female | Reddish | 4 | Native | No | 1:800 | -ve |
130 | 60 | Female | White | 4 | Native | No | 1:1600 | -ve |
Discussion
This is the first study in Bangladesh to investigate any domestic animal for VL infection. Our results showed that cattle produced antibodies which might be due to their exposure to the Leishmania parasite through infected sandfly bites but were unable to produce any infection. The absence of parasite DNA in molecular assays might be due to failure of the parasite to survive or propagate in the host.
Earlier in India, search for possible animal reservoir for VL mostly targeted to dogs based on direct observation of smears for amastigotes from peripheral blood, liver, spleen, and bone marrow [22–24]. Chakravarty et al. surveyed 64 cows along with dog, but could not find any amastigote in the smears [23].
At present, ELISA and DAT are two commonly-used serological methods for screening domestic and wild animals for the detection of anti-Leishmania antibodies. Due to insufficient information and lack of previous investigation in the Indian subcontinent; we adapted a cut-off titer of 1:3200 for DAT which was previously used in Sudan for screening anti-L. donovani antibodies in several domestic and wild species, including cows [14].
The presence of anti-L. donovani antibodies in ELISA and DAT of the cattle serum in our study supports the finding of a previous study in Sudan [14]. In Brazil, anti-Leishmania antibodies were found in domestic swine but were apparently resistant to Leishmania infection which may also occur in the case of cattle [25].
Antibody response in the cattle might also be due to the cross-reacting antibodies inferred by other infections which have been observed previously in human sera. For example anti-Leishmania antibodies were found cross-reactive with tuberculosis, toxoplasmosis, and malaria [26, 27]. However, in this study, no such investigation for cross reactivity was done. The antibodies response in the few positive cattle in our study was quite weak which might be due to undiluted sera used in ELISA.
In a recent study in Nepal, Leishmania DNA was detected in domestic animals, such as goats, cows, and buffaloes, several months after the active transmission season [15]. We could not follow up our study cattle for detection of the parasite DNA in the following months due to limited resources which is a limitation of our study.
Conclusions
Based on the findings of our study, it can be suggested that cattle are not a reservoir host for L. donovani despite its preference by P. argentipes as blood source. However, further studies need to be carried out to investigate the role of other domestic animals in VL epidemiology in this region.
Declarations
Acknowledgements
This study was supported by ICDDR, B and its donors which provide unrestricted support to the Centre for its operations and research. Current donors providing unrestricted support include: Government of the People's Republic of Bangladesh; Canadian International Development Agency (CIDA), Embassy of the Kingdom of the Netherlands (EKN), Swedish International Development Cooperation Agency (Sida), and the Department for International Development, UK (DFID). We gratefully acknowledge these donors for their support and commitment to ICDDR, B's research efforts and activities. The authors also thank Mr. M. Shamsul Islam Khan, Head, Publication Unit, ICDDR, B, for language editing of the manuscript.
Authors’ Affiliations
References
- WHO: Report of the Fifth Consultative Meeting on Leishmania/HIV Co infection. Addis Ababa, Ethiopia: World Health Organization; 2007.Google Scholar
- WHO/TDR: Research to support the elimination of visceral leishmaniasis.Annual Report 2008 World Health Organization; 2009, 27.Google Scholar
- Rijal S, Koirala S, Van der Stuyft P, Boelaert M: The economic burden of visceral leishmaniasis for households in Nepal. Trans R Soc Trop Med Hyg. 2006, 100 (9): 838-841. 10.1016/j.trstmh.2005.09.017.PubMedView ArticleGoogle Scholar
- Das S, Boreham PF, Bhattacharya NC, Sen Gupta PC: Prevalence and blood meal sources of Phlebotomus argentipes in West Bengal in 1972-73. Indian J Med Res. 1976, 64 (9): 1307-1313.PubMedGoogle Scholar
- Mukhopadhyay AK, Chakravarty AK: Bloodmeal preference of Phlebotomus argentipes &Ph. papatasi of north Bihar, India. Indian J Med Res. 1987, 86: 475-480.PubMedGoogle Scholar
- Mukhopadhyay AK, Kumar K, Rahman SJ: Host preference of phlebotomine sandflies in and around Delhi. J Commun Dis. 1987, 19 (4): 408-411.PubMedGoogle Scholar
- Palit A, Bhattacharya SK, Kundu SN: Host preference of Phlebotomus argentipes and Phlebotomus papatasi in different biotopes of West Bengal, India. Int J Environ Health Res. 2005, 15 (6): 449-454. 10.1080/09603120500392525.PubMedView ArticleGoogle Scholar
- Pandya AP: Bloodmeals of phlebotomine sandflies of Surat district (Gujarat state) India. Indian J Med Res. 1985, 81: 46-48.PubMedGoogle Scholar
- Bern C, Courtenay O, Alvar J: Of cattle, sand flies and men: a systematic review of risk factor analyses for South Asian visceral leishmaniasis and implications for elimination. PLoS Negl Trop Dis. 2010, 4 (2): e599-10.1371/journal.pntd.0000599.PubMed CentralPubMedView ArticleGoogle Scholar
- Bern C, Hightower AW, Chowdhury R, Ali M, Amann J, Wagatsuma Y, Haque R, Kurkjian K, Vaz LE, Begum M, Akter T, Cetre-Sossah CB, Ahluwalia IB, Dotson E, Secor WE, Breiman RF, Maguire JH: Risk factors for kala-azar in Bangladesh. Emerg Infect Dis. 2005, 11 (5): 655-662.PubMed CentralPubMedView ArticleGoogle Scholar
- Bern C, Joshi AB, Jha SN, Das ML, Hightower A, Thakur GD, Bista MB: Factors associated with visceral leishmaniasis in Nepal: bed-net use is strongly protective. Am J Trop Med Hyg. 2000, 63 (3-4): 184-188.PubMedGoogle Scholar
- Barnett PG, Singh SP, Bern C, Hightower AW, Sundar S: Virgin soil: the spread of visceral leishmaniasis into Uttar Pradesh, India. Am J Trop Med Hyg. 2005, 73 (4): 720-725.PubMedGoogle Scholar
- Saha S, Ramachandran R, Hutin YJ, Gupte MD: Visceral leishmaniasis is preventable in a highly endemic village in West Bengal, India. Trans R Soc Trop Med Hyg. 2009, 103 (7): 737-742. 10.1016/j.trstmh.2008.10.006.PubMedView ArticleGoogle Scholar
- Mukhtar MM, Sharief AH, el Saffi SH, Harith AE, Higazzi TB, Adam AM, Abdalla HS: Detection of antibodies to Leishmania donovani in animals in a kala-azar endemic region in eastern Sudan: a preliminary report. Trans R Soc Trop Med Hyg. 2000, 94 (1): 33-36. 10.1016/S0035-9203(00)90429-2.PubMedView ArticleGoogle Scholar
- Bhattarai NR, Van der Auwera G, Rijal S, Picado A, Speybroeck N, Khanal B, De Doncker S, Das ML, Ostyn B, Davies C, Coosemans M, Berkvens D, Boelaert M, Dujardin JC: Domestic animals and epidemiology of visceral leishmaniasis, Nepal. Emerg Infect Dis. 2010, 16 (2): 231-237.PubMed CentralPubMedView ArticleGoogle Scholar
- Bern C, Chowdhury R: The epidemiology of visceral leishmaniasis in Bangladesh: prospects for improved control. Indian J Med Res. 2006, 123 (3): 275-288.PubMedGoogle Scholar
- Nicholson MJ, Butterworth MH: A guide to condition scoring of zebu cattle. Agribookstore/Winrock; 1986.Google Scholar
- Harith AE, Kolk AH, Kager PA, Leeuwenburg J, Muigai R, Kiugu S, Laarman JJ: A simple and economical direct agglutination test for serodiagnosis and sero-epidemiological studies of visceral leishmaniasis. Trans R Soc Trop Med Hyg. 1986, 80 (4): 583-536. 10.1016/0035-9203(86)90149-5.PubMedView ArticleGoogle Scholar
- Islam MZ, Itoh M, Mirza R, Ahmed I, Ekram AR, Sarder AH, Shamsuzzaman SM, Hashiguchi Y, Kimura E: Direct agglutination test with urine samples for the diagnosis of visceral leishmaniasis. Am J Trop Med Hyg. 2004, 70 (1): 78-82.PubMedGoogle Scholar
- Cruz I, Canavate C, Rubio JM, Morales MA, Chicharro C, Laguna F, Jimenez-Mejias M, Sirera G, Videla S, Alvar J: A nested polymerase chain reaction (Ln-PCR) for diagnosing and monitoring Leishmania infantum infection in patients co-infected with human immunodeficiency virus. Trans R Soc Trop Med Hyg. 2002, 96 (Suppl 1): S185-189.PubMedView ArticleGoogle Scholar
- Takagi H, Itoh M, Islam MZ, Razzaque A, Ekram AR, Hashighuchi Y, Noiri E, Kimura E: Sensitive, specific, and rapid detection of Leishmania donovani DNA by loop-mediated isothermal amplification. Am J Trop Med Hyg. 2009, 81 (4): 578-582. 10.4269/ajtmh.2009.09-0145.PubMedView ArticleGoogle Scholar
- Bhattacharya A, Ghosh TN: A search for Leishmania in vertebrates from kala-azar-affected areas of Bihar, India. Trans R Soc Trop Med Hyg. 1983, 77 (6): 874-875.PubMedView ArticleGoogle Scholar
- Chakravarty AK, Sanyat RK, Suri JC: Zoonotic reservoir in Indian kala-azar. J Commun Dis. 1979, 11: 219-220.Google Scholar
- Zahar AR: Studies Leishmaniasis, Vectors/Reservoirs and their control in the old world; Part IV. Asia and Pacific. World Health Organization;198087.Google Scholar
- Moraes-Silva E, Antunes FR, Rodrigues MS, da Silva Juliao F, Dias-Lima AG, Lemos-de-Sousa V, de Alcantara AC, Reis EA, Nakatani M, Badaro R, Reis MG, Pontes-de-Carvalho L, Franke CR: Domestic swine in a visceral leishmaniasis endemic area produce antibodies against multiple Leishmania infantum antigens but apparently resist to L. infantum infection. Acta Trop. 2006, 98 (2): 176-182. 10.1016/j.actatropica.2006.04.002.PubMedView ArticleGoogle Scholar
- Badaro R, Eulalio MC, Benson D, Freire M, Miranda JC, Pedral-Sampaio D, Burns JM, David JR, Johnson WD, Reed SG: Sensitivity and specificity of a recombinant Leishmania chagasi antigen in the serodiagnosis of visceral leishmaniasis. Arch Inst Pasteur Tunis. 1993, 70 (3-4): 331-332.PubMedGoogle Scholar
- Burns JM, Shreffler WG, Benson DR, Ghalib HW, Badaro R, Reed SG: Molecular characterization of a kinesin-related antigen of Leishmania chagasi that detects specific antibody in African and American visceral leishmaniasis. Proc Natl Acad Sci USA. 1993, 90 (2): 775-779. 10.1073/pnas.90.2.775.PubMed CentralPubMedView ArticleGoogle Scholar
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