Mobile suitcase laboratory for rapid detection of Leishmania donovani using recombinase polymerase amplification assay
© Mondal et al. 2016
Received: 5 February 2016
Accepted: 5 May 2016
Published: 13 May 2016
Leishmania donovani (LD) is a protozoan parasite transmitted to humans from sand flies, which causes Visceral Leishmaniasis (VL). Currently, the diagnosis is based on presence of the anti-LD antibodies and clinical symptoms. Molecular diagnosis would require real-time PCR, which is not easy to implement at field settings. In this study, we report on the development and testing of a recombinase polymerase amplification (RPA) assay for the detection of LD.
A genomic DNA sample was applied to determine the assay analytical sensitivity. The cross-reactivity of the assay was tested by DNA of Leishmania spp. and of pathogens considered for differential diagnosis. The clinical performance of the assay was evaluated on LD positive and negative samples. All results were compared with real-time PCR. To allow the use of the assay at field settings, a mobile suitcase laboratory (56 × 45.5 × 26.5 cm) was developed and operated at the local hospital in Mymensingh, Bangladesh.
The LD RPA assay detected equivalent to one LD genomic DNA. The assay was performed at constant temperature (42 °C) in 15 min. The RPA assay also detected other Leishmania species (L. major, L. aethiopica and L. infantum), but did not identify nucleic acid of other pathogens. Forty-eight samples from VL, asymptomatic and post-kala-azar dermal leishmaniasis subjects were detected positive and 48 LD-negative samples were negative by both LD RPA and real-time PCR assays, which indicates 100 % agreement. The suitcase laboratory was successfully operated at the local hospital by using a solar-powered battery. DNA extraction was performed by a novel magnetic bead based method (SpeedXtract), in which a simple fast lysis protocol was applied. Moreover, All reagents were cold-chain independent.
The mobile suitcase laboratory using RPA is ideal for rapid sensitive and specific detection of LD especially at low resource settings and could contribute to VL control and elimination programmes.
KeywordsLeishmania donovani Recombinase polymerase amplification assay Suitcase laboratory Visceral leishmaniasis Bangladesh
Leishmania donovani (LD) causes visceral leishmaniasis (VL) in humans, kala-azar in the Indian Subcontinent (ISC), where a VL elimination programme is underway . Individuals who have been infected through the bite of a sand fly, harbor the parasite in mononuclear phagocytic cells and can remain asymptomatic for the rest of their lives, or develop symptomatic VL. If left untreated, VL could be lethal; after treatment, a proportion of subjects develop a cutaneous form known as post-kala azar dermal leishmaniasis (PKDL).
Diagnosis is currently based on the detection of anti-Leishmania antibodies in subjects with clinical symptoms (persisting fever and splenomegaly). Serological assays, e.g. direct agglutination test (DAT) and rK39 dipstick are widely used especially in poor resource settings. DAT is sensitive and specific, but an 8-hour run-time, low reproducibility and challenging quality control are the main drawbacks [2, 3]. In contrast, the rK39 rapid detection assay is very fast (15 min) and easy to use, but its sensitivity and specificity varies [2–6]. In addition, anti-leishmanial antibodies persist for a long time, therefore, current serological tests cannot be used for cure assessment and diagnosis of VL relapse. However, high anti-leishmanial antibody titre before treatment may be useful for prediction of disease progression .
The VL elimination programme currently underway in the ISC relies on identifying and treating VL as early and efficiently as possible so as to reduce morbidity and mortality and at the same time remove sources of further transmission . Detection of the parasite or parasite DNA would greatly improve case management, disease control as well as the investigation of transmission dynamics.
The presence of the parasite can be detected through molecular diagnosis using the real-time polymerase chain reaction (PCR), which is highly sensitive and specific [8–12] but unsuited for implementation at primary and secondary health-care facilities. It must be operated in a well-equipped laboratory by highly-trained personnel and reagents must be kept at -20 °C .
A highly specific and sensitive test would be needed to sustain the long-term current achievements of the VL elimination programme in the ISC . There is therefore, a demand for a simple and rapid molecular assay. The recombinase polymerase amplification (RPA) assay is an isothermal amplification system . The amplification of the DNA in the RPA relies on enzymes and proteins to replace the repetitive cycles of three temperatures (94 °C, DNA denaturation; 50–60 °C, primer annealing; 72 °C extension) in the PCR. In contrast, the RPA reaction carries out at a constant temperature (42 °C) and even using the body heat . In addition, all reagents are cold chain independent and can be kept at 38–40 °C ambient temperature for up to three months without any effect on the assay performance [17–19].
In this study, RPA assay was developed for the detection of the LD and assay sensitivity, specificity and cross-reactivity were studied. To facilitate the use of the developed assay at point of need, two mobile suitcase laboratories were developed. In addition, operational feasibility of the suitcase laboratory using RPA and SpeedXtract in the field was also explored.
Generation of the DNA LD molecular standard
A molecular DNA standard representing 1–310 nt of LD kinetoplast minicircle DNA (kDNA, GenBank accession number: Y11401.1) was synthesized and inserted into pcDNA3.3-TOPO plasmid vector (GeneArt, Invitrogen, Darmstadt, Germany). The plasmid was linearized with BbSl restriction enzyme (New England Biolabs, Frankfurt am Main, Germany). The number of DNA molecules per microliter was measured by the Quant-iT™ PicoGreen® dsDNA Assay Kit (Fisher Scientific GmbH, Schwerte, Germany) and calculated with an equation as described before . A dilution range of 107–101 molecules/μl of the molecular standard was produced to determine the analytical sensitivity of LD RPA assay. The standard was tested using a real-time PCR assay as described previously  applying KAPA SYBR FAST ABI Prism kits (Peqlab, Erlangen, Germany) and on the Stratagene Mx305P device (Agilent, California, USA).
LD RPA assay primers and probe
To select the RPA primers and exo probe combination, which produces the highest LD RPA assay analytical sensitivity, eight forward primers (FPs), nine reverse primers (RPs) and one exoprobe were tested (Additional file 1: Figure S1). All oligonucleotides were produced by TibMolBiol (Berlin, Germany). The RPA assay was performed by using the TwistAmp exo kits (TwistDx Cambridge, UK) as described below.
Analytical sensitivity of the LD RPA assay
Concentrations between 107 and 101 molecules/μl of the DNA molecular standard were used to determine the analytical sensitivity of LD RPA assay in eight replicates. In addition, culture promastigote DNA extracted with QIAamp DNA Blood Mini Kit (Qiagen, Hilden, Germany) was used to determine the analytical sensitivity of the RPA assay. Considering 100 fg of culture DNA equivalents to one parasite , analytical sensitivity was determined from 100 to 1 parasite, where the volume of template DNA in each reaction was 5 μl.
Cross-reactivity, clinical sensitivity and specificity of the LD RPA assay
DNA of pathogens listed in Table 2 were used to determine the assay cross-reactivity. Total of 48 archived DNA samples from VL patients, asymptomatic individuals and PKDL patients were tested by both RPA and real-time PCR assays . All VL patients (N = 23) were either parasitologically confirmed or diagnosed with VL in accordance with Bangladeshi national guidelines . Likewise, all asymptomatic individuals (N = 5) were habitants of VL endemic areas and clinically healthy but positive in Leishmaniasis DAT and rK39 dipstick test. PKDL patients (N = 20) were rK39 test positive with previous history of VL and negative for fungus and leprosy. To determine the specificity of the assay, 48 archived DNA samples including endemic healthy controls (N = 35), non-endemic healthy controls (N = 5) and disease controls (six malaria cases and two TB cases) were also investigated. QIAamp DNA Blood Mini Kit (Qiagen, Hilden, Germany) was used to extract DNA from Buffy coat of VL patients, asymptomatic and control individuals where QIAamp DNA mini kit was used for the skin biopsy from PKDL patients. All VL, PKDL and asymptomatic cases were positive for LD DNA by real-time PCR, while controls (healthy and disease) were negative for rK39, DAT and LD DNA by real-time PCR as described below.
Real-time PCR for Leishmania
Quantitative detection of Leishmania DNA was performed on a Biorad CFX96 icycler system using primers and Taqman probe: 5′-GCG ACG TCC GTG GAA AGA A-3′, 5′-GGC GGG TAC ACA TTA GCA GAA-3′ and (FAM): 5′-CAA CGC GTA TTC CC-3′ (Applied Biosystems Inc., Foster City, CA, USA) targeting the repetitive sequence of L. infantum Genome (77–142 nt of Genbank accession number: L42486.1) by following a previous method . Each reaction was run using a total of 11 μl of PCR mix (Applied Biosystems Inc., Foster City, CA, USA) plus 9 μl of extracted DNA (buffy coat or skin biopsy). Each sample was run in duplicate. However, samples with very late amplification (≥ 40 cycles) were repeated in triplicate.
Mobile suitcase laboratory
In the extraction suitcase, a simple fast lysis protocol (SpeedXtract, Qiagen, Hilden, Germany) was deployed as follows: 500 μl of whole blood was incubated with 1500 μl of the enrichment buffer and 30 μl of the magnetic beads for 3 min at room temperature. The magnetic beads were separated using a magnetic stand and then the supernatant was removed without disturbing the beads. Then the beads were washed twice with 500 μl enrichment buffer. Thereafter, 100 μl of the lysis buffer was added and the mix was incubated at 95 °C for 10 min. The beads were then separated and 5 μl of the supernatant was used in the RPA reaction. The total time needed for the extraction was 20 min.
In the detection suitcase, 5 μl of the RPA primers and probe mix was added to the RPA lyophilized pellet (TwistAmpexo kits, TwistDx, Cambridge, UK) at concentration of 420 nM and 120 nM, respectively. Then 40 μl of rehydration buffer containing 14 mM Mg acetate was added. Finally, 5 μl of template was added. The tube was closed and mixed well before it was placed into the tubescanner (Twista, TwistDx, Cambridge, UK) and incubated for 15 min at 42 °C. The emitted fluorescence signals were measured at 20 s intervals. A combined threshold and first derivative analysis was used for signal interpretation. The total time for RPA reaction including handling was 20 min.
Field feasibility evaluation of suitcase laboratory
Blood samples were collected from seven patients hospitalized at the Surya Kanta Kala-azar Research Center in Mymensingh (Additional file 1: Figure S2). Nucleic acid was extracted from whole blood using the SpeedXtrcat method and RPA test was performed in the field as described above. Concurrently, buffy coats were shipped to the central diagnostic laboratory in the icddr, b, where DNA was extracted from the buffy coat using the Qiagen DNA blood kit and real-time PCR was carried out as described before .
For the LD RPA assay analytical sensitivity using the molecular DNA standard, a semi-log regression analysis and a probit analysis were performed by plotting the RPA threshold time against the number of molecules detected using PRISM (Graphpad Software Inc., San Diego, California) and STATISTICA (StatSoft, Hamburg, Germany), respectively. Sensitivity and specificity were calculated using standard formulas.
The study used archive samples, which were collected through different previous studies with Principal Investigator Dr. Dinesh Mondaland G. M. Khan (PR-13090, PR-13045 and PR-09069). For use of archive samples for eventual future activities on VL, consent from study participants and approval from the Ethical Review Committee of the icddr, b had been obtained.
LD RPA primers and probe sequences
Cross-reactivity investigation for LD RPA assay
Number of isolates
Sample type and reference test
LD RPA assay results
L. donovani MHOM/ET/67/HU3Z18
Reference DNA with concentration of around 40–100 ng/μl
Paul-Ehrlich-Institute, Langen, Germany
L. major MHOM/IL/81/FEBNI
L. aethiopica MHOM/ET/72/L100Z14
L. infantum (50134D) MHOM/TN/80/IPT-1
American Type Culture Collection, Manassas, USA
L. tropica (50129D)
Dept. of Microbiology, University Medical Center Gottingen, Germany
DNA extracted from blood samples of malaria patients. Plasmodium species-specific nested PCR was performed .
DNA extracted from culture
DNA extracted from lymph node aspirate from two extra pulmonary TB patients. Both were positive in culture and IS6110 PCR .
Comparison between real-time PCR and LD RPA assays in detecting LD in 96 samples
Cases (N = 48)
100 % (23/23)
100 % (5/5)
100 % (20/20)
Controls (N = 48)
Endemic healthy control
100 % (35/35)
Non-endemic healthy control
100 % (5/5)
100 % (8/8)
During the field assessment at Surya Kanta Kala-azar Research Centre in Mymensingh (Additional file 1: Figure S2), five samples were positive in both real-time PCR and RPA, while two samples were negative (Additional file 1: Table S2). Using suitcase laboratory, results were produced in 40 min, which included extraction and detection procedures, whereas, real-time PCR was performed in 4 h in a highly equipped laboratory in icddr, b, Dhaka.
The LD RPA assay was designed to amplify 160 nt of the kDNA gene, which is present in a high copy number in LD (~10,000 DNA copies/cell) . The LD RPA assay detected down to 100 DNA copies applying the LD DNA linearized plasmid (Fig. 2), and one LD genomic DNA (Fig. 3). Using 96 buffy coats and skin biopsies collected from VL, asymptomatic and PKDL cases as well as negative control, the LD RPA assays had the same clinical sensitivity and specificity as the real-time PCR  (Table 3). However, the RPA produced results six to nine times faster than the real-time PCR, and does not require the same level of equipment and training.
The most challenging step in the RPA assay development is the design of a primer pair able to amplify a very low DNA copy number [13, 17, 18, 25–28]. Neither a program nor strict rules are available. In this study, 8 FPs and 9 RPs were chosen randomly around the exo probe binding sites (Additional file 1: Figure S1). All oligonucleotides combination failed to reach the needed assay sensitivity except FP3 and RP3 (Table 1). The LD RPA exo probe generating the highest fluorescence signal was placed in the same direction as the RP and has a short 5′ end. The same model was successfully applied in two studies [18, 25], but did not performed well in others [13, 19].
The LD RPA assay did detect L. donovani and other Leishmania spp. (L. major, L. aethiopica and L. infantum). This is due to the fact that the RPA primers and probe are able to amplify and detect target genes containing 5–9 mismatches [25, 29, 30]. A BLAST search revealed an identity between 93 and 100 % of RPA FP3 and RP3 and 88–100 % of the RPA exo probe to sequences of the above mentioned Leishmania species (Additional file 1: Figure S3).
Recently, a RPA assay for the detection of canine VL was developed . The assay amplified both LD and L. infantum. It deployed a lateral flow system to readout the results with naked eyes, which tremendously decreases the assay run costs. Nevertheless, this required additional steps to transfer the amplified product to another tube for dilution and detection, which increased the possibility of cross-contamination and the assay run time . In contrast, our approach depended on a probe system that allowed the amplification and the detection in a single closed tube.
Several loop-mediated isothermal amplification (LAMP) assays were established to identify the Leishmania parasites [33–38]. The LAMP results can be read by naked eye, nevertheless, the LAMP assay requires six primers and no probe system has yet been implemented. Moreover, LAMP produced results in 60 min . In contrast, the RPA assay was very fast (in a maximum of 15 min) and utilized two primers and one probe.
The SpeedXtract represents a promising tool for the nucleic acid extraction at point of need. First it allowed the isolation of leukocytes from the whole blood in 3 min. Then a simple DNA extraction protocol combining a lysis buffer and heat is applied. Moreover, the reagent is stable at room temperature. The SpeedXtract without the enrichment step was previously deployed for Ebola virus RNA extraction . To the best of our knowledge, this is the first report on using it for a parasitic disease.
There are several reasons why we need a test that can detect the presence of Leishmania parasites and can be deployed widely in low-resource settings. Effective case management requires a test that can diagnose VL among other causes of illness (differential diagnosis) and assess as early as possible whether treatment has succeeded or failed (test-of-cure). Effective, sustainable VL control and elimination requires a test that can identify subjects who can transmit the infection as early as possible (even before they become symptomatic) to remove the source of transmission . Especially now that the prevalence of the disease had dropped following the attack phase of the VL elimination programme in the ISC. Such test should be accurate, reproducible, inexpensive and user-friendly.
The current study successfully explored that RPA assay is feasible at field settings to detect leishmaniasis using suitcase laboratory. The selection of suitcase laboratory provided the following advantages: (i) Easy to carry, transport and ship; (ii) Power source from solar panel with power pack; (iii) Easy to be implemented in low resource settings; (iv) A magnetic bead extraction was applied to avoid the creation of aerosols and the use of a high-speed centrifuge; (v) All reagents are cold chain independent; and (vi) A tightened waste container was used, which was autoclaved or incinerated before disposal to avoid contamination to the environment, However, the current cost of the mobile suitcase laboratories and the solar power batteries is 8500 Euro and cost per reaction is six euros inclusive of the controls and the extraction. Lowering the cost will broaden its application in the most affected countries. In addition to diagnosis, integration of an internal positive control and an algorithm for the quantification of number of LD cells will maximize its use as test-of-cure during post-treatment follow-up.
The use of a mobile suitcase laboratory is advantageous for rapid, sensitive and specific detection of LD using SpeedXtract and RPA assay, especially, at low resource settings such as Bangladesh and could contribute to VL control and elimination program. However, before its recommendation for the program, further validation of the LD-RPA assay incorporated in suitcase laboratory through a prospective study is merited.
direct agglutination test
kinetoplast minicircle DNA
loop-mediated isothermal amplification
number of positives (for sensitivity) or negatives (for specificity)
total number of samples
polymerase chain reaction
post-kala azar dermal leishmaniasis
recombinase polymerase amplification
We thank Claus-Peter Czerny, University of Goettingen, Germany for fruitful scientific discussions, Ger van Zandbergen, Paul-Ehrlich-Institute, Langen, Germany and Carsten Lüder, University Medical Center Gottingen, Germany for providing the standard leishmania DNA for the cross-reactivity study. We thank Marvin Kulp of the technical maintenance department of the German Primate Center who helped in assembling the mobile suitcase laboratories and Shereen Petersen for English proofreading. The study was funded by UNICEF/UNDP/World bank/WHO Special Programme for Research and Training in Tropical Diseases (TDR-WHO, project ID: 201293485).
PO is a staff member of the World Health Organization (WHO); the authors alone are responsible for the views expressed in this publication and they do not necessarily represent the decisions, policy or views of the WHO.
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