- Open Access
Development, validation and evaluation of a rapid PCR-nucleic acid lateral flow immuno-assay for the detection of Plasmodium and the differentiation between Plasmodium falciparum and Plasmodium vivax
Malaria Journal volume 11, Article number: 279 (2012)
Molecular tools are very sensitive and specific and could be an alternative for the diagnosis of malaria. The complexity and need for expensive equipment may hamper implementation and, therefore, simplifications to current protocols are warranted.
A PCR detecting the different Plasmodium species and differentiating between Plasmodium falciparum and Plasmodium vivax was developed and combined with a nucleic acid lateral flow immuno-assay (PCR-NALFIA) for amplicon detection. The assay was thoroughly evaluated for the analytical sensitivity and specificity in the laboratory, the robustness and reproducibility in a ring trial and accuracy and predictive value in a field trial.
The analytical sensitivity and specificity were 0.978 (95% CI: 0.932–0.994) and 0.980 (95% CI: 0.924-0.997), respectively, and were slightly less sensitive for the detection of P. vivax than for P. falciparum. The reproducibility tested in three laboratories was very good (k = 0.83). This evaluation showed that the PCR machine used could influence the results. Accuracy was evaluated in Thailand and compared to expert microscopy and rapid diagnostic tests (RDTs). The overall and P. falciparum-specific sensitivity and specificity was good ranging from 0.86-1 and 0.95-0.98 respectively, compared to microscopy. Plasmodium vivax detection was better than the sensitivity of RDT, but slightly less than microscopy performed in this study.
PCR-NALFIA is a sensitive, specific and robust assay able to identify Plasmodium species with good accuracy. Extensive testing including a ring trial can identify possible bottlenecks before implementation and is therefore essential to perform in additon to other evaluations.
The correct and timely diagnosis of life-threatening diseases such as malaria is essential for the initiation of accurate and prompt treatment . However, correct diagnosis of infectious diseases is often difficult in resource-poor settings, resulting in clinical decisions based on presumptive diagnosis . This can lead to unnecessary over-treatment of one disease and under-recognition of another . The diagnosis of malaria is often complicated by the fact that routine microscopy has a relatively low detection limit, is time-consuming and requires experienced microscopists to obtain reliable results . Rapid diagnostic tests (RDTs) could be a good alternative but the detection limit is currently even lower than microscopy, especially when the infecting agent is non-falciparum. RDTs specifically detecting Plasmodium vivax for instance can have a very low sensitivity [5, 6].
Molecular diagnostic tools, such as PCR, are highly sensitive and specific but involve sample processing. The read-out of the assay requires either laborious gel-electrophoresis, which uses toxic products and UV-light or expensive equipment to measure the assay in real time . Simplifying this methodology is thus warranted and has been partly achieved by using, for example, isothermal amplification technologies such as LAMP  or simple and cheap read-out systems, such as nucleic acid lateral flow immuno-assay (NALFIA) [9, 10], which can circumvent the use of electrophoresis or the purchase of expensive real-time PCR machines. NALFIA is analogous to an RDT but instead of detection of antigens it will detect amplified nucleic acids. Like an RDT the sample pipetting is fast, the results can be kept for further reference after the test is performed and the waiting time before the result can be visually read is only 10 minutes without the need of UV light and ethidium bromide.
Essential to the development of a new diagnostic test is determining the accuracy in diagnosing the right condition . Therefore, high sensitivity (the probability of a positive test result for a patient with the disease) and specificity (the probability of a negative test for a patient that does not have the disease) is required . All new diagnostic tests need to be assessed for these characteristics. This entails a comparison with the gold or reference standard that should be infallible. This is difficult in the case of malaria because the obvious reference standards, microscopy and RDT, which are routinely used in the field, are not as sensitive as molecular tools, leading to an underestimation of the specificity of the molecular assay.
Nevertheless, in order to estimate the accuracy of a diagnostic test it has to undergo different testing phases [13, 14]. During the first phase a small study is performed on typical patients with and without the disease of interest, and the analytical sensitivity and specificity is assessed. If it fails this phase than the test is not worth further exploring without significant modifications. During the second evaluation phase in which the diagnostic sensitivity and specificity are assessed, a large number of patients are tested. The patient sample should be representative of the target population. Although these results might give a good reflection of the sensitivity and specificity, it is also essential to study the reproducibility and ruggedness of a test when other operators perform the assay. Although with the ideal test the performance is not operator-dependent, many tests show variation when performed in different laboratories . Having the test performed by different operators and/or different laboratories will reveal whether the test is reproducible or not , and whether a large rollout would be a feasible aim. This can be studied in a so-called ring trial.
This study describes the development of a species-specific PCR combined with NALFIA for the detection of pan-Plasmodium species and the discrimination between Plasmodium falciparum and P. vivax. In addition the test has been evaluated for the accuracy in an exploratory study in the laboratory and thereafter validated in Mea-Sot Thailand for accuracy in the final target population. Reproducibility was assessed by evaluating the assay in a ring trial in three different laboratories that did not participate in the development of the assay.
DNA isolation and PCR
DNA was extracted, with Qiagen DNA mini kit (Qiagen, Germany) according to the manufacturer’s instructions, from all the whole blood samples used in this study. For each sample 200 μl of whole blood was used and the samples were eluted in 200 μl TE buffer. The PCR reaction consisted of primers (Table 1), targeting the 18S gene of Plasmodium and the human housekeeping gene glyceraldehyde 3-phosphate dehydrogenase (GAPDH), which was used as an internal control. For the discrimination of two Plasmodium species, general pan-Plasmodium and specific P. falciparum and P. vivax forward primers were designed. As a reverse primer, a generic primer developed on a conserved region present in all three targets, was used. The PCR reaction with a final reaction volume of 25 μl comprised of 12,5 μl 1X Qiagen Multiplex PCR Master mix (Qiagen, Germany), 200 μM dUTP, 2% DMSO, 1U UNG (Fermentas), primers in the concentration as presented in Table 1, and 2 μl template DNA. The cycling conditions consisted of an nitial step of 10 min at 50°C followed by one step of 15 min at 95°C, 35 cycles of 45 sec at 94°C, 45 sec at 54°C and 60 sec at 72°C and a final step of 10 min at 72°C. For each experiment a blood sample negative for Plasmodium, a sample containing P. falciparum, a sample containing P. vivax and a non-template control of only water were used as control samples.
Nucleic acid lateral flow immuno-assay
A nitrocellulose membrane of 120 mm (Millipore, Amsterdam, The Netherlands) was used for the preparation of the NALFIA. On the nitrocellulose, 0.8 mg/ml anti-Texas Red rabbit IgG fraction (Invitrogen, Paisley, UK), 0.2 mg/ml anti-Digoxigenin polyclonal antibody (Roche Diagnostics, Mannheim, Germany), 0.4 mg/ml anti-dinitrophenyl- rabbit IgG fraction, (Invitrogen, Paisley, UK), and 0.1 mg/ml anti-FITC purified polyclonal antibody rabbit polyclonal IgG, (AbD Serotec, Oxford, UK) were sprayed, all at 0.8 μl/cm and within 4.5 mm distance of each other. A Surewick G041 glass-fibre sample pad (Millipore, Billerica, USA) was used to spray 2.5 μl/cm streptavidin-labelled carbon suspension (three parts streptavidin-labelled carbon and two parts sodium tetraborate buffer solution containing 6.25% sucrose and 6.25% BSA) and attached to the NALFIA stick. The strips were air dried at 37°C, packed in plastic housing and sealed in airtight bags containing silica until further use.
After amplification 5 μl PCR product and 70 μl running buffer (0,1 M borate buffer pH 8.8, 1% BSA and 1% (v/v) sodium azide) were added to the sample pad of the NALFIA and after 10 min the results were read. The NALFIA was considered valid if a black line at the GAPDH position was visible. If in addition to the GAPDH line, the pan line was present then the sample contained Plasmodium DNA. If in addition the P. falciparum line was present then a P. falciparum infection was confirmed. The same held for the P. vivax line in combination with the pan-Plasmodium line. If all four lines were present than it was considered to be a mixed infection. If no line appeared on the GAPDH position, regardless of other lines that might have appeared, the NALFIA test was considered to be a test failure. An example of the different possibilities of the NALFIA outcomes is shown in Figure 1.
Laboratory evaluation PCR-NALFIA
The analytical sensitivity of the PCR-NALFIA test was assessed by using a 5% P. falciparum NF54 ring stage culture (in 5% haematocrit). The cultured parasites were 10-fold diluted with Plasmodium-negative donor blood to obtain malaria parasites dilutions from 0.55% to 5x10-8% in 45% haematocrit. The specificity of the test was determined by analysing malaria positive and negative samples (n = 241) from: i) travellers returning from malaria-endemic areas, diagnosed by an experienced technician by microscopy and/or Plasmodium- specific nested PCR according to[Snounou et al. 16]; ii) from Sudanese patients with a confirmed P. falciparum infection; and, iii) samples provided by the Dutch blood bank which excludes donations of patients who travelled in the past nine months to malaria-endemic areas and can therefore be considered negative for malaria (Table 2).
Inter-laboratory evaluation PCR-NALFIA
In order to assess the inter-laboratory variability of the assay, a diagnostic ring trial was performed. All necessary reagents and 94 processed samples were sent to three laboratories that were not directly involved in the development of the current PCR and NALFIA technology. These materials were accompanied by a protocol on how to perform the assay but no further training was given. The laboratories used their own PCR equipment and the assay was performed by personnel who had previous experience performing PCR. In addition to the patient samples presented in Table 2 two DNA samples of pure P. falciparum culture of 10 and 1 p/μl were provided. The protocol indicated that two non-template controls should be added by the laboratory performing the assay. The technicians performing the assay were blinded as to the contents of the samples and the performance of the other laboratories in the trial.
Field evaluation of PCR-NALFIA, study site and patient description
A prospective study was conducted in the health clinics of Wang Pa and Mae Khon Ken, Mae Sot district, Tak Province, Thailand, which is located on the Thai-Myanmar border. In this hill-forested region, with low year-round transmission and two seasonal peaks from May-September during the rainy season and December-January, the predominant species causing malaria are P. vivax and during the rainy season P. falciparum. Patients were recruited in the malaria clinics of Wang Pa and Mae Khon Ken located around Mae Sot. Samples were transported to the Shoklo Malaria Research Unit (SMRU) in Mae Sot for further processing. Ethical approval for the evaluation in Thailand was obtained from the local ethical review board, Mahidol Oxford Research Unit and the Oxford Tropical Research Committee. Patients visiting the outpatient clinics with the clinical suspicion of uncomplicated malaria, over three years old, and willing to participate in the study, were enrolled after obtaining their informed consent or in the case of minors that of their parents or guardians. Additional inclusion criteria were axillary temperature ≥ 37.5°C or a history of fever in the previous 24 hours.
From each participant, finger prick blood was collected in EDTA tubes (Stastedt, Numbrecht, Germany) for preparation of thin and thick Giemsa-stained microscopy slides, to perform a HRP-2 and PAN pLDH-based RDT and 200 μl of blood was used for DNA isolation. Microscopy was performed according to international and GCP guidelines by local expert microscopists . Parasites were counted against 500 leukocytes at 1,000x magnification. If only one parasite was found after counting of 500 WBC then counting continued until a second parasite was observed with a limit of counting 4,000 WBC. All slides were read by two microscopists and discordant results were read by a third reader. A leukocyte count of 8000/μL was assumed to calculate the parasite density per μl and the final result was the geometric mean of the readings. Peripheral blood was applied to the SD Bio Line Malaria Antigen P.f/Pan POCT RDT (Standard Diagnostics Inc) according to the procedures described by the manufacturer. The PCR-NALFIA was performed as described above. All test operators were blinded to each other’s test results. On the discordant results and a selection of the microscopy negative samples (n = 71) an additional diagnostic nested PCR was performed as described by Snounou et al..
Data from the laboratory evaluation and the ring trial were directly entered into Excel. Data from the field evaluation were collected on separate case record forms and subsequently entered in Excel. Calculations of sensitivity, specificity and agreement between microscopy, RDT and PCR-NALFIA were done using Epi Info version 6.04 (Center for Disease Control and Prevention, Atlanta, GA, USA). For the ring trial analysis a combined kappa was calculated by using the formula for more than two raters and more than two outcomes as described by [Fleiss et al. 19]. Each of the samples was rated into one of the six subtypes (P. falciparum, P. vivax, negative, P. falciparum and P. vivax mixed infection, non-P. falciparum and non-P. vivax infection or water controls) by the three laboratories. Kappa (κ) values express the agreement beyond chance and were calculated with a 95% confidence interval. Kappa was calculated for each of the subtypes separately against an amalgam of the remaining categories. For example, the P. falciparum kappa is the two-rating kappa where P. falciparum is positive and all remaining outcomes are negative. The combined kappa is the appropriately weighted average of the individual kappas. There is considerably more agreement about the rating of samples as being P. falciparum compared to P. falciparum/P. vivax. A ĸ-value  of 0.21-0.60 is a moderate, a ĸ-value of 0.61-0.80 a good and a ĸ-value >0.80 is an almost perfect agreement beyond chance. Kappas were calculated by STATA SE11.2
Analytical performance of the PCR-NALFIA
The analytical sensitivity could only be assessed for P. falciparum as there was no reference sample with P. vivax available with a certified number of parasites. The analytical sensitivity was 1 p/μl for both the Pan-band and the P. falciparum band with the P. falciparum sample. The samples were also once run on agarose gel to confirm the expected amplicon size of both GAPDH and the Plasmodium fragments.
The phase 1 evaluation of 241 samples resulted in three test failures (two in negative controls and one P. falciparum-positive sample), meaning that no GAPDH line could be observed. Of the negative samples, five were found positive by PCR-NALFIA for P. falciparum, of which two were also positive in the pan-Plasmodium line. None of the negative samples reacted with the P. vivax line. All P. falciparum samples reacted with both the pan-Plasmodium and P. falciparum line, including the sample that had no GAPDH line. None of the samples reacted with the P. vivax line. All P. vivax samples were positive for pan-Plasmodium but three failed to react with the specific P. vivax line. None reacted with the P. falciparum line. Of the 18 Plasmodium malariae samples, three were negative and one indicated a P. vivax infection. All Plasmodium ovale samples, including the P. falciparum/P.ovale mixed infections were identified correctly. The P. falciparum/P.vivax mixed infection samples were all positive for pan-Plasmodium and P. falciparum but one failed to detect the additional P. vivax line.
To determine sensitivity and specificity, the test failures were excluded and microscopy results were used as the reference. The overall sensitivity and specificity for the detection of any species through the pan-Plasmodium line in this specific data set was 0.978 (95% CI: 0.932–0.994) and 0.980 (95% CI: 0.924-0.997) respectively. For the detection of P. falciparum through the specific P. falciparum line, the sensitivity and specificity in this set was 1 (95% CI: 0.946-1) and 0.967 (95% CI: 0.921–0.988). The sensitivity of the P. vivax line was lower in this evaluation (0.857 (95% CI: 0.664-0.953)) but the specificity was good (0.995 (95% CI: 0.969-0.999)).
Intra-assay variability between three independent laboratories
Of the 96 samples that were tested by the three different laboratories, 84 were identified correctly by all three laboratories. Table 3 gives an overview of the score of correct answers per individual laboratory. One sample containing P. falciparum was scored as a test failure in all three laboratories. In addition, laboratory 1 identified two negative samples as a P. falciparum infection, one P. vivax sample as negative and another P. vivax sample as a mixed infection with P. falciparum. Laboratory 2 had only two additional misdiagnoses. One negative sample was interpreted as a non-P. falciparum/non-P. vivax sample and one P. vivax sample was interpreted as a mixed infection with P. falciparum, which was the same sample that was misdiagnosed with the same interpretation as laboratory 1. Laboratory 3 scored the least of the three laboratories. Three samples that were positive for either P. falciparum, P. vivax or P. ovale were scored negative. One negative sample was interpreted as positive for P. falciparum, a P. vivax and a P. falciparum sample were both identified as non-P. falciparum/non-P. vivax and a P. falciparum/P. vivax co-infection was interpreted as a P. falciparum mono-infection. Despite these discrepancies, the overall agreement between laboratories and the reference panel was good to almost perfect. The kappa amongst the different laboratories can be found in Table 4. The agreement between the different samples was also good and can be seen for the different species in Table 3. The overall kappa was 0.839. Only the P. falciparum/P. vivax mixed infection agreement is very low but this is caused by the fact that only one sample of this type was analysed.
Field evaluation of the PCR-NALFIA in a malaria-endemic setting
The evaluation of the PCR-NALFIA took place between December 2011 and January 2012. In total, 381 patients were included of which 85 patients were seen in Mae Khon Ken and 296 in Wang Pa. The mean age of the participants was 20.6 years (range four to 63 years), 33% was female and 67% was male, which is representative for the region. In total, 274 of the patients recruited into the study were found to be negative with microscopy, 72 were found to be harbouring P. vivax, (mean parasitaemia 730 p/μl), 32 P. falciparum (mean parasitaemia 5185 p/μl) and three a mixed infection. A complete overview of the results can be found in Table 5. When RDT is compared to microscopy, RDT had four test failures and detected a substantially lower number of P. vivax cases than microscopy (14 of 72 microscopy confirmed P. vivax were missed). The PCR-NALFIA detected more positive samples than were found negative with microscopy. Three were identified as P. falciparum, six were identified as P. vivax and five others as a mixed infection. The 14 samples that were negative for P. vivax with PCR-NALFIA were the same that were negative with RDT. Seven of these samples had a parasitaemia below two parasites/ μl, four samples between four parasites/μl and 10 p/ul and three between 20 p/μl and 32 p/μl. The calculated sensitivity and specificity of the different detection lines of the PCR-NALFIA compared to the different assays can be found in Table 6. When only the microscopy positive samples are compared to the RDT and PCR-NALFIA results and stratified to parasitaemia, it is found that PCR NALFIA is able to reliably detect samples with a parasitaemia of over 50 p/μl whereas RDT is already having problems with identifying some of the samples below 500 p/μl, as can be seen in Table 7. When the discordant results were analysed with a nested PCR, the three PCR-NALFIA positive P. falciparum samples were confirmed (including the RDT positive sample) to be positive for P. falciparum; three of the P. vivax samples were confirmed to contain P. vivax, however the other three were negative; of the mixed infection, two were found negative and three were found to have only P. vivax. Thirteen out of the 14 samples that were identified as P. vivax positive by microscopy but both PCR-NALFIA and RDT negative were positive in the nested PCR. The other sample was negative. In the group of negative samples that were also analysed with the nested PCR, 15 samples (21%) were identified as P. vivax positive and no other species were found.
This paper describes the development of a multiplex PCR assay for the detection and differentiation of malaria parasites combined with NALFIA to enable fast and easy readout of the results. This assay has been shown to be sensitive and specific and the readout with NALFIA is straightforward.
The assay was evaluated in three different phases. First, the analytical sensitivity and specificity was assessed and found to be very good, although the detection of P. vivax was slightly less sensitive than the detection of P. falciparum which is likely caused by the lower parasite densities present in a P. vivax sample.
Next, the robustness, reproducibility and repeatability of the assay was tested in the ring trial. This phase is often not performed in diagnostic test development and evaluation but it can give extremely valuable results. The current trial has shown, for example, that although in general the reproducibility of the assay was acceptable, there were differences in the results. Laboratory 3 failed to correctly identify some of the samples. Although the overall agreement between the laboratories was good, it was striking that laboratory 3 identified more samples as negative or a mono-infection, pointing to a reduced sensitivity of the assay in this laboratory. The exact mechanism behind this reduced sensitivity in this laboratory was not further investigated and can be the result of a variety of factors altough all reagents, samples and materials were provided to the laboratory and were the same as the other laboratories received. It should be noted that this was the only laboratory that performed the amplification on a Biorad-CFX Real-Time PCR machine, whereas the other laboratories used conventional PCR machines. The Real-Time machinery has a variable ramping time which can be installed manually whereas the other conventional PCRs have fixed ramping times and are therefore comparable in this respect. It was however not investigated whether or not the Real-Time PCR machine was the cause of the slightly poorer results but it cannot be excluded. This issue would not have would not have surfaced if a ring trial had not been performed. In all three laboratories and in the field evaluation, use of the NALFIA as a readout system was received enthusiastically by performers and was carried out without any particular difficulties.
In the final field evaluation, the sensitivity, specificity and predictive value of the assay was studied in a moderate transmission area for P. falciparum and P. vivax parasites. In this study the results of PCR-NALFIA were compared to both microscopy and RDT. Although microscopy is often considered to be the gold standard, it is not sensitive enough compared to PCR or other molecular diagnostics and may consequently obscure the results of the specificity of the assay under investigation . RDTs are even less sensitive but were used in this study to compare the performance of the PCR-NALFIA with another assay that is used on a day-to-day basis . Because of these limitations the discordant results were also analysed by a sensitive nested PCR. This study showed that PCR-NALFIA performs very well for the detection of P. falciparum and is as sensitive and specific as microscopy and PCR. The assay was also very sensitive compared to RDT and was able to pick up all samples over 50 parasites/ul that were found positive in microscopy. For P. vivax, the microscopy performed in this study was more sensitive although some samples that were found negative with microscopy were found positive in PCR and confirmed positive with the nested PCR as well. The microscopy performed extremely well in this study and it is therefore essential to mention that the protocol used for slide reading is different from the one that is used as standard in routine care, and which is usually less sensitive.
While it was not observed in the present study, a possible concern might be the risk of contamination when a PCR sample is transferred to the NALFIA device. Altough this could partly be circumvented by performing the PCR set up and amplification in one room and do the read-out in another, a closed system in which no leakage to the environment is possible should be the next step in the development. Another current disadvantage is that this assay relies on PCR technology for amplification, which demands electricity. This does not have to be a problem if the assay is going to be performed in a setting where constant supply of electricity can be guaranteed. However, if one desires to use this assay in more remote settings in which no constant supply of electricity is available, alternative platforms that are less dependent on electricity, such as LAMP  or NASBA , could be considered. Nevertheless, although these assays are generally considered to be sensitive and specific they should be subjected to a thorough analysis on their robustness, reproducibility, repeatability and user-friendliness before implementation can be considered.
The current NALFIA strips were produced by a manufacturer specialized in the production of lateral flow devices and because of the large amount of strips produced the price for the NALFIA strips is around €0,50 cent. The final costs will depend on the quanitity of devices produced. This will also depend on the shelflife of the NALFIA devices. This has not been extensively studied in this study but the devices used were performing well up to a period of 6 months after dispatching at room temperature.
Even though all reagents and materials were provided by the developers of the assay and the technicians that performed the assay, in both the ring trial and laboratory evaluation, had previous experience in molecular techniques, no training on the current protocol was given. This shows PCR-NALFIA is a user friendly procedure that can be performed with no or little extra training.
The assay in its current format, or slightly modified with more sensitive detection of P. vivax, could be an excellent tool for epidemiological studies on prevalence or distribution of parasites. In addition, it could be used as a screening tool at regional level for malaria control programmes especially in countries with declining transmission . Molecular tools have been shown to be especially valuable in areas where there is moderate to little transmission  and PCR-NALFIA may be a straightforward method to implement.
PM coordinatied and and preparated the laboratory and trial work, drafted the protocols, analysed the data and drafted the manuscript. AM participated in the initial test development. LdB prepared the laboratory evaluation and was involved in the single laboratory trial. JF provided technical assistance and prepered the lateral flow devices. JS and LK participated in the field trial and performed expert microscopy of the samples. JV, CvO and RH participated in the ring trial, and critically read the manuscript. BW: perfromed the PCR-NALFIA in the field. SP: provided local coordination and supervision of the fieldwork in Thailand, participated in data collection, entry and analysis of the data and critical reading of the manuscript. HS: Conceived the study and coordinated the Malactres project, drafted the of protocols, and was involved in design, preperation and supervision of laboratory and field trials, Coordinaton of the MALACTRES project. AA: Supervised the initial test development. All authors read and approved the final manuscript.
World Health Organization: Guidelines for the treatment of malaria. 2010, WHO, Geneva, Second
Kyabayinze DJ, Asiimwe C, Nakanjako D, Nabakooza J, Counihan H, Tibenderana JK: Use of RDTs to improve malaria diagnosis and fever case management at primary health care facilities in Uganda. Malar J. 2010, 9: 200-10.1186/1475-2875-9-200.
Ansah EK, Narh-Bana S, Epokor M, Akanpigbiam S, Quartey AA, Gyapong J, Whitty CJ: Rapid testing for malaria in settings where microscopy is available and peripheral clinics where only presumptive treatment is available: a randomised controlled trial in Ghana. BMJ. 2010, 340: c930-10.1136/bmj.c930.
Kahama-Maro J, D'Acremont V, Mtasiwa D, Genton B, Lengeler C: Low quality of routine microscopy for malaria at different levels of the health system in Dar es Salaam. Malar J. 2011, 10: 332-10.1186/1475-2875-10-332.
Harris I, Sharrock WW, Bain LM, Gray KA, Bobogare A, Boaz L, Lilley K, Krause D, Vallely A, Johnson ML, Gatton ML, Shanks GD, Cheng Q: A large proportion of asymptomatic Plasmodium infections with low and sub-microscopic parasite densities in the low transmission setting of Temotu Province, Solomon Islands: challenges for malaria diagnostics in an elimination setting. Malar J. 2010, 9: 254-10.1186/1475-2875-9-254.
Meena M, Joshi D, Joshi R, Sridhar S, Waghdhare S, Gangane N, Kalantri SP: Accuracy of a multispecies rapid diagnostic test kit for detection of malarial parasite at the point of care in a low endemicity region. Trans R Soc Trop Med Hyg. 2009, 103: 1237-1244. 10.1016/j.trstmh.2009.04.011.
Hawkes M, Kain KC: Advances in malaria diagnosis. Expert Rev Anti Infect Ther. 2007, 5: 485-495. 10.1586/14787188.8.131.525.
Lucchi NW, Demas A, Narayanan J, Sumari D, Kabanywanyi A, Kachur SP, Barnwell JW, Udhayakumar V: Real-time fluorescence loop mediated isothermal amplification for the diagnosis of malaria. PLoS One. 2010, 5: e13733-10.1371/journal.pone.0013733.
Posthuma-Trumpie GA, Korf J, van Amerongen A: Lateral flow (immuno)assay: its strengths, weaknesses, opportunities and threats. A literature survey. Anal Bioanal Chem. 2009, 393: 569-582. 10.1007/s00216-008-2287-2.
Noguera P, Posthuma-Trumpie GA, van Tuil M, van der Wal FJ, de Boer A, Moers AP, van Amerongen A: Carbon nanoparticles in lateral flow methods to detect genes encoding virulence factors of Shiga toxin-producing Escherichia coli. Anal Bioanal Chem. 2011, 399: 831-838. 10.1007/s00216-010-4334-z.
Bossuyt PM, Irwig L, Craig J, Glasziou P: Comparative accuracy: assessing new tests against existing diagnostic pathways. BMJ. 2006, 332: 1089-1092. 10.1136/bmj.332.7549.1089.
Sahaa AJ, Hoover DR: “Sensitivity” and “specificity” reconsidered: the meaning of these terms in analytical and diagnostic settings. Ann Intern Med. 1997, 126: 91-94.
Weinstein NA S, Obuchowski M, Lieber L: Clinical evaluation of diagnostic tests. Am J Roentgenology. 2005, 184: 14-19.
Proux S, Suwanarusk R, Barends M, Zwang J, Price RN, Leimanis M, Kiricharoen L, Laochan N, Russell B, Nosten F, Snounou G: Considerations on the use of nucleic acid-based amplification for malaria parasite detection. Malar J. 2011, 10: 323-10.1186/1475-2875-10-323.
World Organization of Animal Health: Principles and methods of validation of diagnostic assays for infectious diseases. Chapter 1.1.4/5. Terrestrial Manual. 2010, Office International des Epizooties, Paris, p1-p18.
Snounou G, Viriyakosol S, Zhu XP, Jarra W, Pinheiro L, Do Rosario VE, Thaithong S, Brown KN: High sensitivity of detection of human malaria parasites by the use of nested polymerase chain reaction. Mol Biochem Parasitol. 1993, 61: 315-320. 10.1016/0166-6851(93)90077-B.
SMRU-Shoklo Malaria Research Unit. 2012,http://www.shoklo-unit.com
World Health Organization: Basic malaria microscopy, Part I Learner's guide. 2010, World Health Organization, Geneva, 2
Fleiss JL, Levin B, Paik MC: Statistical Methods for Rates and Proportions. 2003, Wiley press, New York, 3
Altman DG: Practical Statistics for Medical Reseatch. 1991, Chapman & Hall, London, 611-
Sirichaisinthop J, Buates S, Watanabe R, Han ET, Suktawonjaroenpon W, Krasaesub S, Takeo S, Tsuboi T, Sattabongkot J: Evaluation of loop-mediated isothermal amplification (LAMP) for malaria diagnosis in a field setting. Am J Trop Med Hyg. 2011, 85: 594-596. 10.4269/ajtmh.2011.10-0676.
Schneider P, Wolters L, Schoone G, Schallig H, Sillekens P, Hermsen R, Sauerwein R: Real-time nucleic acid sequence-based amplification is more convenient than real-time PCR for quantification of Plasmodium falciparum. J Clin Microbiol. 2005, 43: 402-405. 10.1128/JCM.43.1.402-405.2005.
malERA consultative group on diagnoses and diagnostics: A research agenda for malaria eradiaction: diagnoses and diagnostics. PLoS Med. 2011, 8: 1000396-
Mens P, Spieker N, Omar S, Heijnen M, Schallig H, Kager PA: Is molecular biology the best alternative for diagnosis of malaria to microscopy? A comparison between microscopy, antigen detection and molecular tests in rural Kenya and urban Tanzania. Trop Med Int Health. 2007, 12: 238-244.
This project was financially supported by the EU funded FP7 project MALACTRES (Multi-drug resistance in malaria under combination therapy: Assessment of specific markers and development of innovative, rapid and simple diagnostics) grant nr 201889. We thank all collaborators of the MALACTRES project for their contribution. We want to specifically thank Dr Colin Sutherland of the London School of Hygiene and Tropical Medicine (UK) and Malaria Reference Laboratory (UK) and Dr Bakri Nour from Wad Medani Teaching Hospital (Sudan) for their kind provision of the blood samples for the laboratory and ring trial evaluation. We are also grateful to the staff and patients of Mae Khon Ken, and Wang Pa malaria clinics and the Shoklo Malaria Research Unit (Thailand) part of Mahidol-Oxford Tropical Medicine Research Unit (MORU) supported by the Wellcome Trust (UK) for their willingness to participate in this trial. We thank Dr Masja Straetmans (Royal Tropical Institute, The Netherlands) for her support in the analysis of the ring trial data.
The authors declare that they have no competing interests.
Authors’ original submitted files for images
Below are the links to the authors’ original submitted files for images.
About this article
Cite this article
Mens, P.F., Moers, A., de Bes, L.M. et al. Development, validation and evaluation of a rapid PCR-nucleic acid lateral flow immuno-assay for the detection of Plasmodium and the differentiation between Plasmodium falciparum and Plasmodium vivax. Malar J 11, 279 (2012) doi:10.1186/1475-2875-11-279
- Shoklo Malaria Research Unit
- Expert Microscopy
- Lateral Flow Device
- Ring Trial