Abstract
Diagnosis of visceral leishmaniasis (VL) through the detection of its causative agents namely Leishmania donovani and L. infantum is traditionally based on immunochromatographic tests, microscopy of bone marrow, spleen aspirates, liver or lymph node and differential diagnosis. While the first process has low specificity, the later one carries the risk of fatal hemorrhage. Over the last decade, multiple Polymerase Chain Reaction (PCR) based diagnosis has been developed using blood and urine sample with a varying degree of sensitivity and specificity, an issue worth improving for precision diagnosis. Earlier, we reported a PCR-based diagnosis of L. donovani in peripheral blood using a novel set of PCR primers with absolute specificity. Using the same set of primers and PCR conditions, here we describe diagnosis of L. donovani from urine, for a non-invasive, rapid and safe diagnosis. Diagnosis of VL was carried out using urine samples collected from clinically diagnosed VL patients (n = 23) of Bangladesh in Real Time PCR. Test results were validated by comparing blood samples from the same set of patients. Sensitivity and specificity of this diagnosis was analyzed using retrospective bone marrow samples, collected earlier from confirmed VL patients (n = 19). The method showed 100% sensitivity in detecting L. donovani in urine and corresponding blood and retrospective bone marrow samples, as well as 100% specificity in control groups. A Real Time PCR-based molecular detection system using urine sample is hereafter presented what could be a, non-invasive approach for VL detection with precision and perfection.
Citation: Rahim S, Sharif MM, Amin MR, Rahman MT, Karim MM (2022) Real Time PCR-based diagnosis of human visceral leishmaniasis using urine samples. PLOS Glob Public Health 2(12):
e0000834.
https://doi.org/10.1371/journal.pgph.0000834
Editor: Om Prakash Singh, Banaras Hindu University, INDIA
Received: June 30, 2022; Accepted: November 28, 2022; Published: December 29, 2022
Copyright: © 2022 Rahim 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 study was financially supported by the University Grants Commission Bangladesh through the University of Dhaka in the form of a grant (Regi: Admin- 3/12247, dated 16 Sep 2021) awarded to MMK. The funder 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.
Introduction
The protozoan parasite Leishmania donovani (LD) is the causative agent for visceral leishmaniasis (VL) or kala-azar (KA), which is a vector-borne disease transmitted by the bite of female sand fly. The parasite exists in two stages to complete its life cycle: Amastigote (developed in human) and Promastigote (in sand fly). The amastigote form residing in the cells of mononuclear phagocytic system (MPS), like macrophage, neutrophil and endothelial cells of human, multiplies by binary fission until the cells of the MPS enlarged. Infected cells are eventually ruptured and the parasites are liberated in the circulation and invade fresh cells; the cycle is repeated until all cells of MPS are affected. Proliferation of MPS cells leads to massive splenomegaly and hepatomegaly. The bone marrow is also involved, resulting in pancytopenia.
Approximately 90% of the 500,000 estimated annual cases of kala azar occur in rural areas of Bangladesh, India, Nepal, Sudan and Brazil [1] whereas Bangladesh, India and Nepal account for 60% of global cases caused by LD. This disease accounts for 40,000 deaths annually [2]. In Bangladesh, 45 out of 64 districts are endemic for VL, while 20 million people are at risk of developing VL [3].
In recent years, Polymerase Chain Reaction (PCR) as well as Real-Time PCR based diagnostic methods have been evaluated for the diagnosis of VL and shown excellent sensitivities and specificities using spleen aspirate, bone marrow, lymph node and blood [4–7]. These processes, however, are invasive and some of them require skilled health personnel to collect samples. Furthermore, possible risk of internal hemorrhage during collection of splenic aspiration or bone marrow biopsy could be lethal for patients. Urine, on the other hand is a non-invasive specimen, which could be a potential source for detection of VL, for it is a systemic and chronic disease associated with acute kidney injury (AKI).
Multiple cases of proximal tubular injury and glomerular inflammation have been reported to be related with VL associated nephropathy [8–12]. It has been postulated that glomerulonephritis occurs due to deposition of immune-complex in kidney. Leishmania bodies in kidney were also detected in light and electron microscopy [13], therefore it is likely to be present in urine.
Given the involvement of VL associated nephropathy, a PCR-based diagnosis of VL caused by L. infantum using urine was developed in Brazil [14, 15]. However, similar strategy is yet to be adopted in Bangladesh, India and other countries of south Asia and south-east Asia for detection of VL caused by L. donovani, a species indigenous in this region [16]. Moreover, PCR-based diagnosis of VL that has been developed using blood and urine samples showed varying degrees of sensitivity and specificity owing to the variation of the PCR techniques (conventional versus Real Time -PCR), DNA extraction method, target Leishmania spp as it diverges from geographical regions, and the set of primers directed to bind to the template Leishmania chromosomes [17]. For example, VL diagnosis using urine in conventional PCR setting showed sensitivity ranging between 25% and 92.8%, while real time PCR based diagnosis showed sensitivity from 47% up to 96.8% [14, 17–20]. Moreover, due to variation in DNA extraction methods detection limit for leishmanial DNA varies and DNA extraction using phenol chloroform showed low reproducibility [5, 21]. Earlier, this lab developed a blood-based method of diagnosing VL using a novel set of primers, MK1 primer pair specific to L. donovani that produced 98% sensitivity and 100% specificity [7]. Here, we took the advantage of using the same set of primers, as it produced profound edge of sensitivity [7], over other sets of primers published in the literature [22, 23]. The suitability of MK1 primer is hereafter justified using urine as sample from patients with VL in both conventional and real time PCR settings, thereby establishing a patient-friendly, non-invasive method of disease diagnosis.
Materials and methods
Ethical clearance and study group
An Ethical clearance from Dhaka Medical College Hospital (DMCH), Dhaka, Bangladesh (reference: Memo No. ERC-DMC/ECC/2021/409, dated 23 Nov 2021), and Bangladesh Medical Research Council (reference number BMRC/NREC/2013-2016/816, dated 8 May 2014) as well as formal written consents from individuals participated in this study were duly obtained at the onset of the study. For participants under 18 years of age, the formal written consent was obtained from the respective parent/ guardian.
Twenty-three patients with clinically diagnosed VL (CDVL) group were enrolled in this study; twenty-one of them were admitted in the DMCH, while the rest two were in Bangabandhu Sheikh Mujib Medical University (BSMMU). Seventeen of them were adult male, five were adult female and one was a male child. Twenty participants were enrolled as healthy control (HC) group; ten each from VL endemic and non-endemic areas. There were nineteen confirmed VL (CVL) patients, and twenty-five patients formed the disease control (DC) group with symptomatic diseases, i.e., tuberculosis (n = 10), malaria (n = 3), and dengue (n = 12) as reported earlier [7] (see the first row of Table 3).
Clinical diagnosis of the patients
Clinical diagnosis of the patients was confirmed by the clinicians at DMCH, and BSMMU, Dhaka, Bangladesh. Patients with clinical signs such as fever, splenomegaly and hepatomegaly symptoms who were admitted in DMCH and BSMMU until March 2022 were confirmed with VL by on-site serology test (rk39-based Immunochromatographic test (ICT)), microscopy of parasitology (observation of amastigote in spleen or bone marrow aspirations), and medical examination by resident clinicians.
Sample collection
Urine.
First morning urine samples were collected from all CDVL patients (n = 23) and stored at 4°C before DNA extraction was done within an hour of sample collection. Briefly, 50 mL of urine were collected from each individual in a 100 mL plastic container (Falcon, USA) and were centrifuged at 12,000 ×g for 5 minutes; then the pellet was suspended in phosphate buffer saline (PBS) for DNA extraction. Urine (n = 20) was also collected from healthy control (HC) group consisting of healthy individuals of non-endemic (Dhaka, n = 10) and endemic areas (n = 10).
Blood.
2 ml venous blood samples were collected in K3 EDTA Tube (13x75mm, Purple Cap, 2mL) from the same set of CDVL patients (n = 23) from where urine samples were collected. On the other hand, venous blood was also collected from both volunteers of HC group (n = 20), and patients with symptomatic diseases similar to VL of disease control group (n = 25; 10, 3 and 12 patients diagnosed for tuberculosis, malaria and dengue respectively). Blood sample processing was conducted within an hour of collection until then samples were stored at 4°C. To separate buffy coat from whole blood, blood was centrifuged at 300 xg for 10 minutes. Supernatant plasma above the buffy coat layer was removed and the layers of buffy coat followed by erythrocytes underneath (to a depth of about 1 mm) were collected using a Pasteur pipette.
Bone marrow. Retrospective bone marrow samples collected from the CVL (n = 19) patients participated in an earlier study [7] were considered for the current analyses.
Positive control. L. donovani DNA, obtained from culture positive promastigote was used as the positive control.
DNA extraction
Total DNA was extracted from urine using QIAamp® DNA Mini Kit (Qiagen, Germany) following manufacturer’s instructions. In order to extract DNA from blood samples, 50μL of blood buffy coat was homogenized with 1 mL of Tween 20, nonidet P-40, NaOH, Tris pH 7.2 (TNNT) buffer and 10μL of a proteinase K solution (containing 320μL of the enzyme/mL) in a 1.5 mL micro-centrifuge tube. Then it was incubated for 3 hours at 56°C followed by an incubation at 72°C for 10 min. The homogenate was then kept at 37°C overnight before 200μL of a phenol–chloroform–isoamyl alcohol mixture (25:24:1 by volume) were added. After vigorous shaking, the mix was centrifuged (10,000 ×g for 10 min), and then the DNA in the aqueous layer was separated, and precipitated with 400μL cold absolute ethanol. The pellet was re-suspended in 50μL double-distilled water before storing at 4°C.
Conventional PCR reaction
Five microliters of purified DNA extracted from both blood or urine samples was used as template in polymerase chain reactions (PCR). The templates were probed using the same MK1F/R primers (Forward primer 5’-CCCAAACTTTTCTGGTCCTC-3’, Reverse primer 5’-GAGCCGATTTTTGGCATTT-3’) which were designed to amplify a 102 bp fragment of leishmanial kinetoplast DNA for the detection of VL [7]. The reaction was performed with an initial denaturation step at 95°C for 10 min, followed by 40 cycles of amplification (95°C/30 sec, 45°C/30 sec, 72°C/30 sec). The PCR products were analyzed by electrophoresis on a 1.2% (w/v) agarose (Thermo Scientific, Mol Bio Grade, USA) gel, containing ethidium bromide (0.5 mg/mL in TBE buffer), 0.04 M Tris-borate and 0.001M EDTA; thereafter photographed under UV illumination using Gel documentation system (Alpha Imager HP System Versatile Gel Imaging, Santa Clara, CA, USA).
Real-Time PCR reaction
Real-time PCR based detection of VL was conducted using the MK1F/R primers in the ABI PRISM 7000 system (Applied Biosystems, USA). For each 20μL reaction mix a 5μL sample of DNA, 1μL of 10 μmol/L of each primer MK1F and MK1R [7], 10μL GoTaq™ qPCR Master Mix (containing BRYT Green® Dye having spectral properties similar to those of SYBR® Green I Promega™, USA), and 3μL of nuclease-free water were added. The reaction was performed with an initial denaturation step at 95ᴼC for 10 min, followed by 40 cycles of amplification (95°C/30 sec, 60°C/30 sec). Non-template control (NTC) and positive control were included. ABI PRISM software (version 1.1) was used for result analysis. Melt curve pattern for the PCR amplicons was produced using a temperature gradient from 60°C to 95°C. The melt pattern was analyzed for the pick at 82±2°C, the theoretical melting temperature of the 102 bp-long amplicon of MK1 primer pair.
Sensitivity, linearity and reproducibility of Real Time PCR assay
A known six 10-fold serial dilutions of DNA (1 ng to 10fg/μL) extracted from in vitro cultured promastigotes of L. donovani corresponding to 10,000 to 0.1 parasites per microliter was used to determine the minimal number of parasites that could be calibrated by the assay. Each reaction contained 1μL of parasite DNA. Three replicates of six 10-fold DNA concentrations were tested in a single run for intra-assay validation. For inter assay validation, similar dilutions were made and three independent runs were performed. The coefficient of variation (CV; represented as the ratio of mean to standard deviation, SD) measures the assay’s variability. Melt curve analysis was conducted to evaluate the analytical specificity of real-time PCR products.
Limit of detection for urine and blood samples
The possible PCR inhibitory effect of biological samples, urine and blood used for VL diagnosis, was analyzed to determine the limit of detection. 200μL of urine collected from one VL negative (in PCR based diagnosis) participant living in non-endemic area was mixed with in vitro cultured promastigotes of L. donovani to a concentration of 100 parasite bodies per microliter. DNA extracted from that spiked urine and three 10-fold serial dilutions of that DNA (10pg to 10fg/μL) corresponding to 100 to 0.1 parasites per microliter were used to determine the minimal number of parasites that could be in urine and assess the inhibitory effect of urine on the standard detection limit of the real time PCR assay.
In order to measure the limit of detection from blood samples, 200μL blood buffy-coat collected from the participant who contributed urine for the same analysis was mixed with in vitro cultured promastigotes of L. donovani to a concentration of 100 parasite bodies per microliter. The DNA was extracted from the spiked blood buffy-coat using previously described phenol chloroform method, thereafter was subjected to determination of limit of detection after making three 10-fold serial dilutions of that DNA (10pg to 10fg/μL) corresponding to 100 to 0.1 parasites per microliter by real time PCR assay (Including the primary DNA extract).
Each real time PCR reaction contained 1μL of DNA extract from either spiked urine or spiked blood buffy-coat. Each reaction was replicated for two times.
Statistical analysis
Online tool Vassar Stats was used to calculate the statistical analyses at 95% confidence interval (CI). The sensitivity and the specificity of the primer pairs were calculated according to the following statistical formulas:
Sensitivity = [a/ (a + c)] × 100
Specificity = [d/ (b + d)] × 100
where a, b, c and d represent numbers of true positive, false positive, false negative, and true negative samples respectively.
Result
Clinical history of the patients
The clinically diagnosed VL patients (n = 23) were 16 to 86 years old (median 36 year). They were admitted with a history of 1 to 2.5 months (median 1.6 month) of fever before hospitalization. 72% of the patients had splenomegaly and 63% of them had hepatomegaly while all of them were reported to have anemia as well as weight loss. There was no post kala azar dermal leishmaniasis (PKDL) case in the study. Again, no patients took anti- leishmanial drug during the episode of VL. Samples were collected from CDVL patients admitted either at DMCH or BSMMU. The respective institutions used their standard protocol for the diagnosis of VL in CDVL patients depending on the condition of the patients, for example, microscopic examination of bone marrow (n = 1) and splenic aspirate (n = 3), and rk39 ICT test (n = 19) in addition to the on-site medical examination by the physicians. The subsequent Real Time PCR-based molecular detection was thereafter conducted using urine and blood of the clinically diagnosed VL patients.
On the other hand, DNA extracted from bone marrow samples (n = 19), collected from CVL patients participated in a preceding study [7] preserved in DNA bank of Fermentation and Enzyme Biotechnology Laboratory (FEBL), Department of Microbiology, University of Dhaka were taken into consideration for diagnosis by Real Time PCR.
Conventional PCR
DNAs collected from the urine specimens of the 23 clinically diagnosed patients, produced the amplicon of 102 bp in polymerase chain reactions when probed with MK1F/R primers (Fig 1). The finding was no different when DNAs collected from the buffy coat preparations of the corresponding patients were used as template in a similar set of PCR reaction. The diagnostic sensitivity of VL using urine as specimens was measured 100% (95% Cl, 85.19–100%) when compared to conventionally-used specimen and the peripheral blood samples (Table 3). Importantly, none of the 20 control urine samples collected from healthy individuals produced the amplicon, indicating 100% specificity of the analyses (Table 3). The success of qualitative measurement of sensitivity and specificity prompted us to estimate limits of detection of pathogen loads using quantitative Real Time PCR analyses.
Fig 1. Detection of LD kinetoplast from urine of CDVL patients using novel MK1F/R primers in conventional PCR.
The PCR-amplified bands using novel MK1F/R primers of 102 bp fragment of leishmanial kinetoplast DNA were produced from 22 urine samples of CDVL patients labeled U1 through U22. Amplicons were separated on a 2% agarose gel; PTC was positive template control containing DNA of cultured LD; NTC was negative template control.
Real-Time PCR
Analytical sensitivity, linearity, reproducibility of Real time PCR assay.
With discernible amplification and melt curve around 81°C, the real-time PCR assay detected as little as 10 fg of LD genomic DNA per reaction, which corresponds to 0.1 parasite (Fig 2). The standard curve produced by gradual dilution of parasite DNA over a 6-log range and cyclic threshold (Ct) values formed a linear relation, with an R2 of 0.994 and PCR efficiency of 94% (Fig 2B). The absence of Ct values in the non-template control validated the specific response of the reaction mix. For six distinct concentrations, the intra assay coefficient of variation (CV) of Ct values were, 0.030%, 0.057%, 0.122%, 0.166%, 0.122% and 1.140% respectively (Table 1). More variability was observed with smaller amount of parasite DNA. Inter assay variation of Ct values for the same dilution series in two independent runs was used to test the assay’s reproducibility. The coefficients of variation between assays were determined to be 1.672%, 1.645%, 2.371%, 2.576%, 1.735% and 3.4% percent, showing strong reproducibility (Table 1).
Fig 2. Analytical sensitivity and detection limit of VL diagnosis using Real Time PCR.
Amplification curves are shown for DNA extracted from 6 log serially diluted L. donovani culture, ranging from 1×104 to 1×10-1 parasite per microliter (A). A standard curve is constructed based on the mean of Ct values plotted against serial dilutions containing corresponding L. donovani DNA (B). Each point represents the Ct value of an individual sample and the plot represents a linear function (R2 = 0.994). Melt curve of amplification product showing peak near 80.78°C (C).
Limit of detection in urine and blood sample
The limit of detection was estimated as little as 10fg DNA or 0.1 parasite per microliter of suspension in PBS. This estimate was found consistent for both urine and blood samples, collected from a single VL negative participant, spiked with in vitro-cultured promastigotes of L. donovani (Table 2). Furthermore, for both spiked urine and blood samples, the melt curve was consistent around 81°C. Variability was insignificant among the respective Ct values for all four dilutions of the spiked urine and blood samples (Table 2).
Clinical sensitivity and specificity of Real time PCR based diagnosis of VL
Presence of L. donovani was evaluated by determination of the Ct and estimation of melting temperature (Tm) using Real-time PCR method. Here, DNAs collected both from the urine of all of the 23 clinically-confirmed patients produced amplification with MK1F/R primers rendering sensitivity 100% (95% Cl, 85.19–100%) (Table 3). Detectable amplifications were found with Ct values between 15 to 28 (Fig 3A). This finding was no different when DNAs, collected from buffy coat preparations of blood specimens from corresponding patients were utilized. Retrospective DNAs extracted from bone marrow of 19 VL-confirmed patients also produced amplification with Ct values between 9 to 22, producing an absolute sensitivity, 100% (95% Cl, 82.35–100%) (Fig 3A). The detected Tm values of all types of samples was near 81°C which is close to the theoretical melting temperature of the 102 bp amplicon, 82°C, therefore validating the specificity.
Fig 3. Ct value in CDVL and CVL patients and parasite load in CDVL patients.
Ct value in urine from CDVL (n = 23), in blood from respective CDVL (n = 23) and in bone marrow from CVL (n = 19) patients, each point indicates data collected from individual patient (A). Parasite burden in urine and blood samples of CDVL (n = 23) patients are illustrated (B).
Parasite load in two different biological samples of CDVL patients was compared and it was found that parasite load in urine, estimated 1 to 329 promastigote/mL, was comparatively lower than that of blood 49 to 5532 promastigote/mL for the same set of patients(Fig 3B).
No amplification was observed in both blood and urine samples of individuals, collected from all endemic and non-endemic healthy control with undetected Ct value in real time PCR. Again, no cross reaction was observed with DNA extracted from blood of malaria, tuberculosis and dengue patients indicating 100% (95% Cl, 82.35–100%) specificity of this diagnosis (Table 3).
Discussion
Visceral leishmaniasis is one of the major health issues of tropical and sub-tropical countries like Bangladesh, India, Nepal, Brazil and Iran. However, rapid and accurate diagnosis of the agent is a major concern in controlling this disease. The microscopic detection of amastigote of Leishmania donovani in aspirates from lymph node, bone marrow and spleen are the gold standard for the diagnosis, and hold a sensitivity of 53%–65%, 53%–86% and 93%–99% respectively [24]. Although the sensitivity of the bone marrow/ splenic smear is high, collection of these specimens is not only painful but also poses a threat of fatal hemorrhage for the patients.
Alternative serodiagnosis of leishmaniasis (based on antibody detection) including ELISA showed different sensitivity and specificity depending on the type, source, and purity of the antigens. Some Leishmania antigens have shown cross reactivity with antigens of other microorganisms [24–26]. However, detection of antibody (IgG) in urine of patients has been used for the VL diagnosis with a sensitivity and specificity up to 98% and 95% respectively, with notable limitations: such as, false positive reactions in endemic areas, and inability to distinguish between current, subclinical, or past infections [20, 21, 27, 28].
Polymerase chain reaction (PCR)-based diagnostic methods for the detection of VL have shown excellent sensitivities and specificities using various biological samples: spleen aspirate, blood, lymph node and bone marrow [22, 29–31]. A blood-based method of diagnosis of VL using novel primer MK1F/R specific for L. donovani showed 98% sensitivity and 100% specificity [7]. Different studies showed that SYBR green Real time PCR-based diagnosis of VL targeting its minicircle DNA demonstrated sensitivity of 79% to 95.7% in blood samples [32, 33]. On the other hand, TaqMan probe based real time PCR produced up to 100% sensitivity in assays targeting genomic DNA from blood samples [34].
The use of urine as specimens has gained usefulness because of its non-invasive nature, minimal risk of blood-borne infections, and easy collection method, especially when infants are concerned. Urine-based direct anti-globulin test with the antibody (sensitivity 90.7%), and urine ELISA (sensitivity 93.3%) were reported as useful alternatives [35, 36]. PCR based diagnosis of VL using urine sample produced promising results with varying degrees of sensitivity and specificity [17]. Here, we compared a real time PCR-based diagnosis of VL caused by L. donovani using urine with that of blood and bone marrow. Primarily, the diagnosis of VL was supported by (1) the observation of amastigote in bone marrow aspirations, (2) response of rk39-ICT in serology, and (3) clinical examination by resident physicians, thereby confirming the diagnosis. In order to develop a PCR-based molecular detection method for VL that would ensure rapidity and precision of the diagnosis, urine samples of the participating patients were used as specimen; there they produced (a) bands of interest with a size of 102 bp in the electrophoretogram in conventional PCR (Fig 1) (b) the amplification with Ct values ranging 18 to 28 in a Real time -PCR (Fig 2A) after necessary extraction of DNAs. Detectable amplification was also present when analyzing the blood samples of corresponding patients, and in the retrospective 19 bone marrow samples of confirmed VL patients in the conventional PCR as well as real time PCR settings (Table 3).
In this study, Real Time PCR assay was able to detect 0.1 parasite per reaction using either urine or blood samples with a detectable melt curve. The limit of detection of this analysis is comparable and, in some cases, better than other currently available dye and probe-based Real Time PCR, while most of them were studied for VL diagnosis from blood or other more invasive biological samples [33, 34, 37, 38]. It is noticeable that the diagnosis using urine showed 100% sensitivity which is same as it showed using blood and bone marrow specimens. And this MK1(F/R) primer-based diagnosis of VL in both conventional and Real Time PCR setting using urine as well as blood showed superior sensitivity and specificity, in compared to other PCR based diagnosis of VL. In addition, this Real Time PCR assay has the potential to quantify the parasite bodies in the VL patients.
Although the target of the MK1F/R primer is the kinetoplast DNA with a tendency to vary among the parasite cells, Ct values among the replicates for particular dilutions remained consistent with very low intra-assay and inter-assay CV indicating a strong correlation between parasite load and respective Ct values (Table 2). Furthermore, the Ct values from the spiked urine and blood buffy coat also followed the earlier Ct values resulted from reproducibility assay for respective parasitic load (Table 3). The limit of detection of this real time PCR-based detection from both urine and blood was as little as 0.1 parasite body per microliter sample. Among the VL patients, parasite load was significantly higher in blood than the corresponding urine samples of the patients (Fig 3B). This comparatively low parasite load in urine was due to the fact that renal filtration system could be compromised due to immunological reactions that lead discharge of parasites or infected macrophages harboring parasites in urine [8, 9, 12, 15]. Contrarily, leishmanial promastigote infects the macrophages (in liver and spleen) and Kupffer cells (in liver) and multiply there that are eventually released in blood making their presence more prominent in blood than that of urine [39].
The road map of World Health Organization (WHO) for neglected tropical diseases (NTD) aims to eradicate VL including PKDL from 75 endemic countries by 2030 by emphasizing (a) research on the relationship among the human, vector, parasite and reservoir, (b) development of more specific and user-friendly diagnostic test, and (c) introduction of faster, more effective, safer, cost effective treatment for the VL patients worldwide [40]. Due to its commendable sensitivity and specificity for urine samples, Real-Time PCR-based diagnosis of VL using MK1 primer can be a suitable detection method to replace blood or more invasive specimens such as bone marrow or spleen. Furthermore, when compared to conventional and nested PCR-based techniques, the ease of one-step molecular detection of RT-PCR reduces work load for the pathologists, thereby fulfilling the patient-friendly diagnostic requirement to achieve the WHO objective. This method can also be used in assessing the response to therapy, monitoring parasite kinetics, infection dynamics and epidemiological survey.
The cohort of this study for diagnosis of VL from urine samples was small (n = 23), therefore further study is necessary to ascertain the degree of sensitivity and specificity of the diagnostic procedure. Moreover, the average admittance of the studied patients in the hospital was 1.7 months after the onset of illness (range 1 to 2.5 months). Therefore, the length of this diagnostic strategy beyond 2.5 months’ post-infection needs to be evaluated. Nevertheless, this is the first report of its kind in Indian sub-continent to use urine as a clinical specimen for detection of L. donovani and its impact in global public health in eradicating this NTD is significant.
Conclusion
Invasive specimens like bone marrow, splenic aspiration or blood could be substituted by non-invasive specimen, urine to score the infection with L. donovani in patients by Real Time PCR without compromising the diagnostic efficiency of VL in Bangladesh, and this success is worth investigating in other VL endemic areas of the world.
Acknowledgments
We are thankful to Professor Dr Anowara Begum and Dr Zenat Zebin Hossain, Department of Microbiology, University of Dhaka for providing technical support to conduct Real-Time PCR analysis.
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