Open Access

Country-wide assessment of the genetic polymorphism in Plasmodium falciparum and Plasmodium vivax antigens detected with rapid diagnostic tests for malaria

  • Natacha Mariette1,
  • Céline Barnadas1,
  • Christiane Bouchier2,
  • Magali Tichit2 and
  • Didier Ménard1Email author
Contributed equally
Malaria Journal20087:219

https://doi.org/10.1186/1475-2875-7-219

Received: 21 July 2008

Accepted: 28 October 2008

Published: 28 October 2008

Abstract

Background

Rapid diagnostic tests (RDTs) are becoming increasingly indispensable in malaria management, as a means of increasing the accuracy of diagnosis. The WHO has issued recommendations, but the selection of the most suitable RDT remains difficult for users in endemic countries. The genetic variability of the antigens detected with RDTs has been little studied, but may affect the sensitivity of RDTs. This factor has been studied by comparisons between countries at continental level, but little information is available concerning antigen variability within a given country.

Methods

A country-wide assessment of polymorphism of the PfHRP2, PfHRP3, pLDH and aldolase antigens was carried out in 260 Plasmodium falciparum and 127 Plasmodium vivax isolates, by sequencing the genes encoding these antigens in parasites originating from the various epidemiological strata for malaria in Madagascar.

Results

Higher levels of polymorphism were observed for the pfhrp2 and pfhrp3 genes than for the P. falciparum and P. vivax aldolase and pldh genes. Pfhrp2 sequence analysis predicted that 9% of Malagasy isolates would not be detected at parasite densities ≤ 250 parasites/μl (ranging from 6% in the north to 14% in the south), although RDTs based on PfHRP2 detection are now recommended in Madagascar.

Conclusion

These findings highlight the importance of training of health workers and the end users of RDTs in the provision of information about the possibility of false-negative results for patients with clinical symptoms of malaria, particularly in the south of Madagascar.

Background

Since the emergence and spread of Plasmodium falciparum parasites resistant to inexpensive anti-malarial drugs, such as chloroquine (CQ) and sulphadoxine-pyrimethamine (SP), routine malaria case management has changed in endemic countries, such as Madagascar. Malaria diagnosis in these areas – particularly in zones not well covered by healthcare facilities – was entirely based on clinical examination, with CQ widely administered for any fever with no obvious alternative cause [13]. Since the introduction of more effective, more expensive anti-malarial drug combinations, such as artemisinin combination therapy (ACT), the WHO recommends the establishment of an accurate biological diagnosis before treatment and the withdrawal of presumptive anti-malarial treatment for all patients other than children under the age of five years in hyperendemic areas. This change in medical practice is now a public health priority in Africa, ensuring that effective anti-malarial drugs are administered only to the patients who need them and limiting the unnecessary use of inappropriate treatment, exposure to potential drug toxicity and the development of drug resistance.

The detection of Plasmodium species by the examination of blood films under a microscope remains the gold standard method for malaria diagnosis. However, this method, despite its simplicity and low cost, is not available everywhere. In peripheral health centres, in particular, there may be no appropriate microscope in working order or a lack of consumables, such as slides or Giemsa stain, or the staff may not have received appropriate training [4]. The development of alternative diagnostic tests for malaria, such as rapid diagnostic tests (RDTs), over the last ten years has made it possible to extend biological diagnosis to remote areas with few resources. These lateral-flow immunochromatographic tests detect specific antigens produced by malaria parasites and are rapid and simple to carry out, requiring no electricity or specific equipment [57]. A large number of branded RDT products are now available commercially (86 RDT products from 28 manufacturers), but all are based on the same principle and only three groups of antigen are detected. Most products detect P. falciparum-specific proteins, either P. falciparum histidine-rich protein 2 (PfHRP2) or P. falciparum lactate dehydrogenase (Pf-pLDH). Some detect both falciparum-specific and pan-specific antigens (aldolase or pan-malaria pLDH), distinguishing non-falciparum infections from P. falciparum or mixed infections.

Increase in the funding of malaria control has resulted in the National Malaria Control Programmes (NMCPs) of many endemic countries considering the possible use of RDTs in health facilities. The choice of an appropriate RDT is based on a number of factors, including sensitivity and specificity, stability, ease of use, cost, the prevalence of the various species infecting humans (choice between RDT detecting only P. falciparum or both P. falciparum and non-falciparum infections) and the format of the RDT. However, many factors, relating to either the parasite or the user, may affect the performance of RDTs for malaria [8, 9]. Diversity in the genes encoding the proteins detected by the RDT may be a particularly important parasite factor. This has been demonstrated for PfHRP2, for which extensive diversity has been shown to affect the detection limits of RDTs based on PfHRP2 detection [10, 11]. However, the degree of antigen variation has recently been shown to be limited for pLDH and parasite aldolase [12, 13], suggesting that antigen polymorphism is unlikely to be responsible for sensitivity variation.

This study, designed to guide the NMCP in Madagascar in its choice of RDT for malaria, had the following objectives: (i) to assess the diversity of the pfhrp2 (and pfhrp3), pldh and aldolase genes in P. falciparum and P. vivax isolates from the various epidemiological strata for malaria in Madagascar and (ii) to determine the potential effect of this diversity on the performance of RDTs for malaria.

Methods

Study sites and parasite isolates

Two hundred sixty P. falciparum and one hundred twenty seven Plasmodium vivax isolates from 16 sites throughout Madagascar were collected in 2006 and analysed. These samples included 160 P. falciparum and 55 P. vivax isolates obtained from febrile inpatients at ten district hospitals and identified by microscopy. A further 172 samples (100 P. falciparum and 72 P. vivax) were collected from febrile outpatients attending six primary health centres. These patients tested positive for malaria with RDTs based on the detection of Plasmodium-specific lactate dehydrogenase (pLDH) (OptiMAL-IT™, DiaMed AG©, Cressier sur Morat, Switzerland). The diagnosis was confirmed by microscopy. These additional samples were not used for assessment of the genetic diversity of Plasmodium lactate dehydrogenase. All blood samples were stored dry spots on filter paper. The geographic distribution of the samples is shown in Figure 1.
Figure 1

Geographic distribution of the 387 samples (260 P. falciparum and 127 P. vivax ) collected in 2006 at 16 sites throughout Madagascar.

DNA extraction

DNA was extracted from blood spots, using Instagene® Matrix resin (BioRad©, Marnes la Coquette, France), according to the manufacturer's instructions. The identification of parasite species was confirmed by real-time PCR, using species-specific primers, as previously described by de Monbrison [14], and a protocol adapted for use with the RotorGene® 3000 thermocycler (Corbett Life Science®, Sydney, Australia).

Amplification by polymerase chain reaction

For P. falciparum, PCR amplification was carried out in a final reaction volume of 55 μl containing DNA template, primers (0.2 μM for each primer), dNTPs (Eurobio© 360 μM for each dNTP), 2.5 mM MgCl2 and 2.5 U FIREPol (Solis Biodyne©). The primers were designed to amplify exon 2 of the Pfhrp2 gene (PfHRP2-R and PfHRP2-F) and the Pfhrp3 gene (HRP3-R1 and HRP3-F2), exon 2 of the Pf-aldolase gene (Pf aldolase R1 and Pf aldolase F1) and the Pf-lactate dehydrogenase gene (PfLDH-R1 and PfLDH-F1). The primer sequences are shown in Table 1. PCR amplification conditions were identical for all four genes: denaturation at 94°C for 5 min, followed by 45 cycles of 94°C for 30 s, 57°C for 40 s and 72°C for 90 s, with a final extension phase at 72°C for 10 minutes.
Table 1

PCR primers, amplicon sizes and accession number of reference sequences used in the study.

PCR primers named

PCR primers sequence 5' to 3'

Target gene

Amplicons size (bp)

GenBank accession number of reference sequences

    

Nucleotide

Protein

PfHRP2-R

TTAATGGCGTAGGCAATGTG

P. falciparum histidine-rich protein II gene, exon 2

905

M13986

AAA51639

PfHRP2-F

TGTGTAGCAAAAATGCAAAAGG

    

HRP3-R1

TGGTGTAAGTGATGCGTAGT

P. falciparum histidine-rich protein III gene

546

AF202093

AAF14632

HRP3-F2

AAATAAGAGATTATTACACGAAAG

    

Pf aldolase R1

TTTCCTTGCCATGTGTTCAA

P. falciparum aldolase gene, exon 2

924

J03084

AAA29716

Pf aldolase F1

AGCAGATGTTGCCGAAGAAT

    

PfLDH-R1

TTTCAGCTATGGCTTCATCAAA

P. falciparum lactate dehydrogenase gene

922

DQ825436

ABH03417

PfLDH-F1

GCACCAAAAGCAAAAATCGT

    

Pvald PF

CCACTGGATCCGAATATAAA

P. vivax fructose 1,6-bisphosphate aldolase gene

1091

AF247063

AAK43741

Pvald PR

CTTTTCGTAAAGGGATGCT

    

Pvald NF

CCTCAAACTACCCGCAGAAG

 

994

  

Pvald NR

GGAGTTCGCTTCTGCTCTCT

    

Pvldh PF

GTAGAGGCAGGTGAACACTC

P. vivax L-lactate dehydrogenase gene

1063

DQ060151

AAY59419

Pvldh PR

TCCTTTTAGTCTCCGCAAC

    

Pvldh NF

AACCCAAAATTGTGCTCGTC

 

900

  

Pvldh NR

CGTCGAACTTGGTCTTCTCC

    

Plasmodium vivax DNA was amplified by nested PCR. The outer PCR was carried out in a final volume of 20 μl containing DNA template, 0.25 μM of each primer, 2.5 mM MgCl2, 200 μM of each dNTP (Eurobio©) and 1 U of FIREPol (Solis Biodyne©). The inner PCR was performed in a final reaction mixture of 55 μl containing PCR amplicons, 0.27 μM of each primer, 2.5 mM MgCl2, 360 μM of each dNTP (Eurobio©) and 2.5 U of FIREPol (Solis Biodyne©). The primer sequences used to amplify the P. vivax fructose 1,6-bisphosphate aldolase gene (outer primers, Pvald PF and Pvald PR; inner primers, Pvald NF and Pvald NR) and P. vivax L-lactate dehydrogenase gene (outer primers, Pvldh PF and Pvldh PR; inner primers, Pvldh NF and Pvldh NR) are shown in Table 1. After denaturation at 94°C for 4 minutes, the DNA was subjected to 40 cycles of 94°C for 20 s, 57°C for 20 s and 72°C for 80 s, with a final extension phase at 72°C for 10 minutes, for the outer PCR. Similar conditions were used for the inner PCR, but with different hybridization (58°C for 20 s) and elongation (72°C for 70 s) temperatures. Positive and negative controls were included in all assays (from the Malaria Research Reference Reagent Resource Center, MR4/ATCC, Manassas, Virginia: HRP II, MRA-67; HRP III, MRA-68, genomic DNA from P. falciparum 3D7, MRA-102G and genomic DNA from P. vivax ONG, MRA-341G).

Direct sequencing of PCR products

PCR products were visualised by agarose gel electrophoresis and purified by filtration through polyacrylamide P-100 Gel (Bio-Gel P-100, BioRad®, Marnes-la-Coquette, France) in 96-well plates (Millipore®, St. Quentin en Yvelines, France). Sequencing reactions were performed with BigDye Terminator chemistry (BigDye v 3.1 Terminator, Applied BioSystem®, Courtaboeuf, France) and a GeneAmp-9700 sequencer (Applied BioSystem®, Courtaboeuf, France). Sequencing was carried out with 10 μl of 0.3 mM EDTA par well, using an ABI 3700 automatic DNA sequencer (Applied BioSystems®, Courtaboeuf, France).

Data analysis

Electrophoregrams were visualised and analysed with CEQTM 2000 Genetic Analysis System software (Beckman Coulter TM). Sequences of insufficient quality were either resequenced or rejected. Amino-acid sequences of the corresponding proteins were deduced from the nucleotide sequences obtained. Nucleotide and amino-acid sequences were compared with the reference sequences in Table 1, using Bio Edit Sequence Alignment Editor Software [15]. For P. falciparum histidine-rich proteins 2 and 3, the amino-acid repeat was identified by numerical code (1–18), as described by Baker et al[10].

Statistical analysis

Based on the results of the analysis, isolates from the various sites were grouped into three distinct geographical regions: the North (Antsiranana, Sambava, Antosohihy, Mahajanga, Maevatanana and Sainte Marie), the Centre (Tsiroanomandidy, Miandrivazo, Mahitsy and Moramanga) and the South (Fianarantsoa, Manakara, Ihosy, Toliara and Ejeda).

The predictive model developed by Baker et al. was used to assess whether an isolate would be detected, if present at a density of ≤ 250 parasites/μl, by a RDT detecting PfHRP2 [10]. PfHRP2 sequences were classified into four groups as a function of the number of type 2 × type 7 repeats: group A (very sensitive) if the PfHRP2 sequence contained a more than 100 type 2 × type 7 repeats, group B (sensitive) if the number of type 2 × type 7 repeats was between 50 to 100, group C (non sensitive) if there were < 43 repeats and "borderline" group if the number of repeats was between 44 and 49.

Differences in the presence/absence of amino-acids repeats in isolates from different geographical areas were assessed by carrying out χ2 tests, and differences in the mean number of amino-acid repeats between the three regions were assessed for each type of repeat, using the Kruskall-Wallis test (H test). P values < 0.05 were interpreted as indicating statistically significant differences.

Results

Polymorphisms in PfHRP2

For the 260 samples collected, 229 PCR pfhrp2 fragments were successfully amplified. These fragments ranged in size from 435 to 927 bp, giving proteins of 145 to 309 amino acids. Thirteen of the 14 different amino-acid repeats previously identified were detected [10]. Two hundred twenty one unique PfHRP2 sequences were identified, 213 of which were found in only one isolate and eight of which were found in two isolates. All PfHRP2 sequences had a similar structure: the type 1 repeat at the start (100% of the sequences), the central motif with the type 7, 8, 2, and 7 repeats combination (66.3% of the sequences) and the type 12 repeat at the end (100% of the sequences). Some repeats were observed in all PfHRP2 sequences (types 1, 2, 6, 7 and 12), whereas others were not observed (repeat 9) or were found in only a few sequences (repeat 8: 97.6%; repeat 3: 92.7%; repeat 10: 89.1%; repeat 5: 83.1%; repeat 4: 24.1%; repeat 13: 9.6%; repeat 14: 8.4% and repeat 11: 0.4%). No differences in the presence/absence of each repeat were found between the three geographic regions (P > 0.05). Further details are provided in Table 2.
Table 2

Distribution of amino-acid repeats in PfHRP2 and PfHRP3 from parasites collected throughout Madagascar in 2006.

No. of amino acid repeats in PfHRP2 and PfHRP3

Region and City

 
  

North

     

Centre

   

South

    

Total

  

ATS

SBV

ATH

MJG

MAE

STM

TDD

MIA

MHT

MOR

FNR

MNK

IHO

TLR

EJE

 

1

AHHAHHVAD

1–5

1–5

1–6

1–5

1–5

2

1–5

1–4

1–3

1–4

2–4

3

1–4

1–4

1–4

1–6

1

AHHAHHVAD

1

1–2

1–3

1–3

1

1

1–3

1–3

1–2

1

1–2

1

1–4

1

1

1–4

2

AHHAHHAAD

8–16

11–13

10–14

4–15

8–14

14

10–14

11–13

11–12

10–13

8–15

12

8–14

7–14

7–15

4–16

3

AHHAHHAAY

0–2

1–2

1–2

0–2

0–2

0

1–2

1–2

1–2

1–2

1–2

0

1–2

1–3

0–3

0–3

4

AHH

0–1

0–1

0–1

0–3

0–2

0

0–1

0–1

0–1

0–1

0

1

0

0–1

0–1

0–3

4

AHH

1

1

1–2

1

1

1

1

1

1

1

1

1

1

1

1

1–2

5

AHHAHHASD

0–1

1

0–3

0–1

0–1

1

0–2

0–2

1

0–1

0–3

0

0–2

1–2

0–2

0–3

6

AHHATD

3–5

3–5

2–5

2–7

2–6

2

2–8

2–6

3–5

3–8

1–3

3

1–3

2–4

2–5

1–8

7

AHHAAD

2–10

4–7

4–11

3–8

4–8

6

3–9

3–8

5–8

3–10

4–13

6

5–10

4–9

3–8

2–13

7

AHHAAD

1

1

1

1

1

1

1

1

1

1

1

1

1

0–1

1

0–1

8

AHHAAY

1–2

1–2

1–2

1–2

1–2

1

0–2

0–2

1–2

0–2

0–2

3

0–2

1–2

1–2

0–2

9

AAY

0

0

0

0

0

0

0

0

0

0

0

0

0

0

0

0

10

AHHAAAHHATD

0–2

0–2

1–3

1–3

1–2

2

0–2

0–2

2–3

1–2

0–2

1

1–2

0–2

0–2

0–3

11

AHN

0

0

0

0–1

0

0

0

0

0

0

0

0

0

0

0

0–1

12

AHHAAAHHEAATH

1

1

1

1

1

1

1

1

1

1

1

1

1

1

1

1

13

AHHASD

0–1

0–2

0–1

0

0–1

0

0–1

0–1

0

0–1

0

0

0–1

0

0–1

0–2

14

AHHAHHATD

0–2

0

0–1

0–1

0–1

0

0–1

0–1

0–1

0–1

0

0

0–1

0–1

0–1

0–2

15

AHHAAY

1

1

1

1

1

1

1

0–1

1

1

1

1

1

1

1

0–1

16

AAY

8–14

8–13

7–13

9–13

8–18

10–14

10–14

10–16

8–14

8–15

8–14

15

10–14

8–15

7–14

7–18

17

AHHAAAHHATD

1–8

5–9

5–8

4–7

5–8

4–8

5–7

3–7

5–10

0–7

4–10

6

4–8

4–6

3–8

0–10

18

AHN

1–3

1–4

1–3

1–4

1–3

2–3

1–3

1–3

2

0–3

2

2

1–2

1–3

2–3

0–4

Significant differences between the number of repeats as a function of geographic region were seen for repeats 5 and 6: isolates from the South had significantly larger numbers of type 5 repeats than isolates from the North and Centre and fewer type 6 repeats than isolates from the North and Centre (Table 3).
Table 3

Comparison of the mean number of each type of repeat in PfHRP2 and PfHRP3 from parasites from different geographic areas.

 

PfHRP2 sequences

PfHRP3 sequences

Type of repeats

Total (n = 229)

North (n = 90)

Centre (n = 81)

South (n = 58)

P

Total (n = 237)

North (n = 90)

Centre (n = 84)

South (n = 63)

P

 

mean

SD

mean

SD

mean

SD

mean

SD

 

mean

SD

mean

SD

mean

SD

mean

SD

 

1

2.6

1.2

2.7

1.4

2.3

1.0

2.66

1.17

0.58

1.1

0.4

1.1

0.4

1.1

0.4

1.2

0.5

0.70

2

12.0

1.8

12.1

2.1

12.1

1.1

11.5

2.3

0.81

         

3

1.4

0.6

1.2

0.7

1.5

0.5

1.5

0.6

0.15

         

4

0.3

0.5

0.3

0.6

0.3

0.5

0.1

0.4

0.47

1.0

0.1

1.0

0.1

1.0

0

1.0

0

0.36

5

0.9

0.6

0.8

0.5

0.9

0.4

1.3

0.7

0.03

         

6

3.4

1;2

3.5

1.1

3.8

1.4

2.7

0.8

0.01

         

7

6.0

2.0

6.0

1.9

6.1

1.7

6.2

2.3

0.73

1.0

0.1

1.0

0

1.0

0

0.98

0.14

0.31

8

1.1

0.5

1.3

0.4

1.1

0.4

1.3

0.6

0.23

         

10

1.5

0.8

1.6

0.7

1.6

0.8

1.4

0.8

0.71

         

13

0.3

0.9

0.2

0.4

0.04

0.2

0,0

0,0

0.08

         

14

0.1

0.3

0.1

0.4

0.1

0.3

0.1

0.3

0.8

         

15

         

1.0

0.1

1.0

0

1.0

0.1

1.0

0

0.43

16

         

11.4

1.8

11.2

1.5

11.5

1.9

11.4

1.8

0.73

17

         

5.8

1.3

5.7

1.3

5.7

1.3

6.0

1.3

0.68

18

         

2.1

0.5

2.1

0.6

2.1

0.5

2.0

0.4

0.61

Based on the model of Baker et al, the frequency of non sensitive isolates (Group C, not detected for parasitaemia ≤ 250 parasites/μl) were predicted to be 9%. No significant differences were found between the three regions in the frequency of the four groups of Baker's model (P > 0.05) (Table 4).
Table 4

Prediction of RDT detection sensitivity based on the regression model of Baker et al (1).

Region of Madagascar

No. of type 2 × type 7 repeats goup (%)

 

Group A

Group B

"Borderline" Group

Group C

Total

North

11 (12)

65 (72)

9 (10)

5 (6)

90

Centre

4 (5)

57 (70)

12 (15)

8 (10)

81

South

7 (12)

36 (62)

7 (12)

8 (14)

58

Total

22 (10)

158 (69)

28 (12)

21 (9)

229

Polymorphisms in the PfHRP3 gene

For PfHRP3, 238 PCR fragments were successfully amplified. They ranged in size from 405 to 720 bp and from the corresponding protein sequences were 135 to 240 amino acids long. Seven of the eight previously described amino-acid repeats were identified [10]. One hundred five unique PfHRP3 sequences were identified: 60 were observed only once, 25 were observed twice, four sequences were shared by three or seven isolates, three sequences were found in four, five and twelve isolates and one sequence was present in six, eight and eleven isolates. All PfHRP3 sequences started with the type 1 repeat and ended with a combination of the type 17 and type 4 repeats.

All repeats found in Madagascar were observed in all PfHRP3 sequences (types 1, 4, 7, 15, 16, 17, 18). No differences in the presence/absence of each repeat were found between the three geographic regions (P > 0.05). Further details are provided in table 2. No significant difference in the number of repeats was observed between the different geographic regions (Table 3).

Polymorphisms in the aldolase gene

Comparisons of 240 P. falciparum aldolase gene sequences obtained from 260 isolates collected throughout Madagascar showed a high level of conservation. Only four single nucleotide polymorphisms (SNP) were observed in six isolates (Table 5). The two parasites with the SNP at nucleotide 815 (amino-acid change at codon 104: H to R) originated from the North (Antsohihy and Maevatanana), whereas the two parasites with the SNP at nucleotide 1404 (amino-acid change at codon 300: H, basic polar amino acid to Q, neutral polar amino acid) originated from the North (Antsiranana) and South (Ejeda). The other two SNPs found in one isolate originated from the South: Ihosy for the SNP at nucleotide 1314 (non synonymous change) and Ejeda for the SNP at nucleotide 1417 (amino-acid change at codon 305: T, neutral polar amino acid to A, neutral non-polar amino acid).
Table 5

SNPs and amino-acids changes in aldolases and pLDHs in P. falciparum and P. vivax isolates collected in Madagascar in 2006, from different geographic areas.

Genes

SNP (bp position and change)

Amino acid change (aa position and change)

Frequency No (%)

P. falciparum aldolase

815 (CAC to CGC)

104 (H to R)

2 (0.8)

 

1314 (CCA to CCC)

synonymous change

1 (0.4)

 

1404 (CAC to CAG)

300 (H to Q)

2 (0.8)

 

1417 (ACC to GCC)

305 (T to A)

1 (0.4)

P. vivax aldolase

510 (TCC to TCA)

synonymous change

1 (0.9)

 

651 (TTA to TTG)

synonymous change

43 (39.1)

P. falciparum LDH

73 (CAG to AAG)

25 (Q to K)

1 (0.7)

 

814 (GAT to AAT)

272 (D to N)

10 (7.3)

P. vivax LDH

168 (ATG to ATA)

56 (D to N)

1 (0.9)

 

225 (AAG to AAA)

synonymous change

84 (75.7)

 

405 (ATC to ATT)

synonymous change

2 (1.8)

 

498 (GTC to GTT)

synonymous change

1 (0.9)

 

544 (GTT to ATT)

182 (V to I)

1 (0.9)

 

627 (GTG to GTC)

synonymous change

32 (28.8)

 

687 (GCC to GCT)

synonymous change

23 (20.7)

For the 110 P. vivax aldolase gene sequences, only two synonymous changes were observed. The SNP at nucleotide 510 were found in one isolate from the Centre (Tsiroanomandidy) whereas the SNP at nucleotide 651 was observed in 43 isolates from the three regions (Table 5).

Polymorphisms in the pLDH gene

Two SNPs were observed among the 137 DNA sequences obtained from the 160 P. falciparum isolates. The SNP at nucleotide 73 (amino-acid change at codon 25: Q, neutral polar amino acid to A, basic polar amino acid) was found in one isolate from Tsiroanomandidy. In addition, 10 isolates displayed a change of nucleotide at position 814 with respect to the reference sequence, resulting in an amino acid change (D, acidic polar amino acid to N, neutral polar amino-acid). These isolates came from the Centre (Mahitsy and Tsiroanomandidy) and the South (Fianarantsoa and Tulear) (Table 5).

Greater diversity in the aldolase gene was observed for P. vivax, with seven different nucleotide changes, including two non-synonymous amino-acid changes. Three synonymous amino-acid changes were frequent and found in all three geographic regions (nucleotide changes at nucleotides 225, 627 and 687). The other four nucleotide changes were rare. The change at nucleotide 405 was displayed by two isolates, one from Miandrivazo and one from Maevatanana, and the change at nucleotide 168 (amino acid change from V to I, two neutral non polar amino acids) was displayed by one isolate from Ejeda. The other two changes were observed in two isolates from Miandrivazo: at nucleotide 168 (amino-acid change from D, acidic polar amino acid to N, neutral polar amino acid) and at nucleotide 498 (Table 5).

Discussion

With the abandon of the inexpensive anti-malarial drug treatments, such as chloroquine, and the use of ACT as a first-line treatment, parasitological confirmation of suspected cases of malaria has become essential. RDTs are now indispensable tools in malaria management, particularly in countries with endemic malaria in which health structures are under-equipped. The WHO has issued some recommendations, but the choice of RTD remains difficult for most users in endemic countries [16, 17]. Indeed, in addition to traditional considerations, such as the Plasmodium species to be detected, the stability of storage and use conditions, ease of use and cost, other technical aspects must be taken into account. One of the most important, but least studied of these factors is genetic variability of the antigens detected by the antibody component of the RTD. Indeed, very few data are currently available, and the available data relate only to continental level [1013]. There is, therefore, clearly a need for more data on pLDH and aldolase antigen variation and the geographic extent of HRP2 variation, especially at local level.

This study provides the first country-wide evaluation of genetic polymorphism for the P. falciparum and P. vivax antigens detected by RDTs for malaria, these two species being the principal species of Plasmodium species found in Madagascar [1820].

Consistent with previous reports [10], the PfHRP2 antigen (and the PfHRP3 antigen) was found to be highly diverse in parasite isolates throughout Madagascar. However, No significant differences, other than the number of repeats for repeats 5 (AHHAHHASD) and 6 (AHHATD), were found in the PfHRP2 and PfHRP3 sequences in the three distinct geographic regions. The sequences obtained were compared with others from around the world [10]. Malagasy HRP2 sequences had certain characteristics in common with African isolates, particularly those from Cameroon (presence of repeats 11, 13 and 14), and with Asian/Pacific isolates, especially those from Thailand (presence of repeats 13 and 14), the Philippines (presence of repeat 11), Papua New Guinea (presence of repeat 14) and the Solomon Islands (presence of repeats 11 and 14), probably reflecting the diversity of populations currently living in Madagascar but originating from Africa, India, Asia, the Middle East and Europe [21].

Finally, Baker's regression model showed that only 91% of the P. falciparum parasites were likely to be detected by RDTs based on HRP2 detection at parasite densities ≤ 250 parasites/μl. We found that the predicted prevalence of parasites undetectable at densities ≤ 205 parasites/μl ("non-sensitive" parasites) was intermediate between that in Asia-Pacific (mean of 23%, range from 17% in South-East Asia to 33% in Papua New Guinea) and that in Africa or South America (0%). We also found that the prevalence of non-sensitive isolates in Madagascar was higher in the South (14%) than in the North (6%), the Centre having an intermediate prevalence (10%). However, this trend was not statistically significant (P < 0.17). One of the major issues linked to the high prevalence of non-sensitive strains in southern Madagascar – an epidemic-prone area – is the high proportion of individuals with low levels of immunity in this region and likely to present clinical symptoms even with a parasitaemia below 250 parasites/μl, a level not generally considered life-threatening. The use of RTDs based on PfHRP2 detection would probably give false negative results in 10% to 20% of cases, leaving patients untreated and therefore at risk of developing severe complications. Indeed, parasitaemia undetectable with RDTs might well occur among the non-immune tourists visiting Madagascar, who would then probably go on to develop clinical symptoms on their return to Europe.

Unlike PfHRP2 (and PfHRP3), the P. falciparum and P. vivax aldolase and pLDH genes appear to be highly conserved among the Malagasy isolates sequenced, confirming published data [12, 13]. Indeed, for the aldolase gene, none of the P. vivax samples displayed an amino-acid change and only three previously undescribed amino-acid changes were identified for P. falciparum samples (at codons 104, 300 and 305). Similarly, we observed only four amino-acid changes in the pLDH gene, two in P. falciparum isolates (at codons 25 and 272) and two in P. vivax samples (at codons 56 and 182). Most P. vivax isolates displayed nucleotide differences with respect to the sequence of the reference strain used: 39.1% of Malagasy isolates displayed a change at nucleotide 651 with respect to the Belem strain aldolase gene sequence (accession no. DQ060151), and 75.7% displayed a change at nucleotide 225, 28.8% at nucleotide 627 and 20.7% at nucleotide 687, with respect to the WDK strain pLDH gene sequence (accession no. AF247063). There are two possible explanations for this difference: sequencing errors for the reference strains used in this study or a specific feature of the Malagasy isolates, these SNPs having never been described before.

Conclusion

The findings of the present study confirm previous data concerning the greater polymorphism of PfHRP2 and PfHRP3 antigens than of P. falciparum and P. vivax aldolase and pLDH antigens. Based on analysis of the PfHRP2 sequences from Madagascar, we predict that 9% of the Malagasy isolates would not be detected at densities ≤ 250 parasites/μl, despite the recommendation to use RDTs based on PfHRP2 detection in the health facilities of the 111 sanitary districts. Thus, in countries using this type of RDT for PfHRP2 sequence detection, efforts should be made to determine more accurately the prevalence of non-sensitive parasites. The results of this study suggest that the National Malaria Control Programme in Madagascar should train its healthcare staff and the end-users of RDTs to provide information concerning the possibility of false-negative results for patients with clinical symptoms of malaria, particularly in South Madagascar. RDTs based on pLDH detection may also be a useful alternative to HRP2-based RDTS, despite their lower sensitivity [22] and stability [23].

Nucleotide sequence accession numbers

The nucleotide sequences reported here have been deposited in the GenBank database under accession numbers EU589688 to EU589767 for P. falciparum hrp-2 sequences, EU589768 to EU589942 for P. falciparum hrp-3 sequences, EU589943 to EU589946 for P. falciparum aldolase gene sequences, EU589947 to EU589948 for P. falciparum pLDH sequences, EU589951 to EU589957 for P. vivax pLDH sequences and EU589949 to EU589950 for P. vivax aldolase gene sequences.

Notes

Declarations

Acknowledgements

The authors thank the Ministry of Health of Madagascar for allowing us access to malaria patients and the patients for participating in the study.

This work was supported by grants from the Genomics Platform, Pasteur Génopôle, Pasteur Institute, France. The collection of samples was supported by the Global Fund project for Madagascar round 3 (Community Action to Roll Back Malaria, Grant number: MDG-304-G05-M) and the World Bank (Project: Cresan 2, No. 196-SANPF/DGADS/UGP/BCP-CRESAN-2).

Authors’ Affiliations

(1)
Malaria Research Unit, Institut Pasteur de Madagascar
(2)
Plate-forme Génomique, Institut Pasteur de Paris

References

  1. Chandramohan D, Jaffar S, Greenwood B: Use of clinical algorithms for diagnosing malaria. Trop Med Int Health. 2002, 7: 45-52. 10.1046/j.1365-3156.2002.00827.x.View ArticlePubMedGoogle Scholar
  2. Kallander K, Nsungwa-Sabiiti J, Peterson S: Symptom overlap for malaria and pneumonia-policy implications for home management strategies. Acta Trop. 2004, 90: 211-214. 10.1016/j.actatropica.2003.11.013.View ArticlePubMedGoogle Scholar
  3. Mwangi TW, Mohammed M, Dayo H, Snow RW, Marsh K: Clinical algorithms for malaria diagnosis lack utility among people of different age groups. Trop Med Int Health. 2005, 10: 530-536. 10.1111/j.1365-3156.2005.01439.x.PubMed CentralView ArticlePubMedGoogle Scholar
  4. Reyburn H, Mbatia R, Drakeley C, Carneiro I, Mwakasungula E, Mwerinde O, Saganda K, Shao J, Kitua A, Olomi R, Greenwood BM, Whitty CJ: Overdiagnosis of malaria in patients with severe febrile illness in Tanzania: a prospective study. BMJ. 2004, 329: 1212-10.1136/bmj.38251.658229.55.PubMed CentralView ArticlePubMedGoogle Scholar
  5. Bell D, Peeling RW: Evaluation of rapid diagnostic tests: malaria. Nat Rev Microbiol. 2006, 4: S34-38. 10.1038/nrmicro1524.View ArticlePubMedGoogle Scholar
  6. Moody A: Rapid diagnostic tests for malaria parasites. Clin Microbiol Rev. 2002, 15: 66-78. 10.1128/CMR.15.1.66-78.2002.PubMed CentralView ArticlePubMedGoogle Scholar
  7. Wongsrichanalai C: Rapid diagnostic techniques for malaria control. Trends Parasitol. 2001, 17: 307-309. 10.1016/S1471-4922(01)01925-0.View ArticlePubMedGoogle Scholar
  8. Bell D, Wongsrichanalai C, Barnwell JW: Ensuring quality and access for malaria diagnosis: how can it be achieved?. Nat Rev Microbiol. 2006, 4: S7-20. 10.1038/nrmicro1525.View ArticlePubMedGoogle Scholar
  9. Bell D, Wongsrichanalai C, Barnwell JW: Ensuring quality and access for malaria diagnosis: how can it be achieved?. Nat Rev Microbiol. 2006, 4: 682-695. 10.1038/nrmicro1474.View ArticlePubMedGoogle Scholar
  10. Baker J, McCarthy J, Gatton M, Kyle DE, Belizario V, Luchavez J, Bell D, Cheng Q: Genetic diversity of Plasmodium falciparum histidine-rich protein 2 (PfHRP2) and its effect on the performance of PfHRP2-based rapid diagnostic tests. J Infect Dis. 2005, 192: 870-877. 10.1086/432010.View ArticlePubMedGoogle Scholar
  11. Lee N, Baker J, Andrews KT, Gatton ML, Bell D, Cheng Q, McCarthy J: Effect of sequence variation in Plasmodium falciparu m histidine-rich protein 2 on binding of specific monoclonal antibodies: Implications for rapid diagnostic tests for malaria. J Clin Microbiol. 2006, 44: 2773-2778. 10.1128/JCM.02557-05.PubMed CentralView ArticlePubMedGoogle Scholar
  12. Lee N, Baker J, Bell D, McCarthy J, Cheng Q: Assessing the genetic diversity of the aldolase genes of Plasmodium falciparum and Plasmodium vivax and its potential effect on performance of aldolase-detecting rapid diagnostic tests. J Clin Microbiol. 2006, 44: 4547-4549. 10.1128/JCM.01611-06.PubMed CentralView ArticlePubMedGoogle Scholar
  13. Talman A, Duval L, Legrand E, Hubert V, Yen S, Bell D, Le Bras J, Ariey F, Houze S: Evaluation of the intra- and inter-specific genetic variability of Plasmodium lactate dehydrogenase. Malar J. 2007, 6: 140-10.1186/1475-2875-6-140.PubMed CentralView ArticlePubMedGoogle Scholar
  14. de Monbrison F, Angei C, Staal A, Kaiser K, Picot S: Simultaneous identification of the four human Plasmodium species and quantification of Plasmodium DNA load in human blood by real-time polymerase chain reaction. Trans R Soc Trop Med Hyg. 2003, 97: 387-390. 10.1016/S0035-9203(03)90065-4.View ArticlePubMedGoogle Scholar
  15. Hall T: BioEdit: a user-friendly biological sequence alignment editor and analysis program for Windows 95/98/NT. Nucl Acids Symp Ser. 1999, 95-98.Google Scholar
  16. World Health Organization: Interim notes on selection of type of malaria rapid diagnostic test in relation to the occurrence of different parasite species. Guidance for national malaria control programmes. Accessed 21 March 2008. 2005, [http://www.wpro.who.int/NR/rdonlyres/CF152D7C-25BA-49E7-86D2-DBEE4E5B5974/0/INTERIMNOTESONMALARIARDTS_RBM_final2_rev3.pdf]Google Scholar
  17. World Health Organization WPRO: Procurement and use of Malaria Rapid Diagnostic Tests. Fact Sheet for GFATM. Accessed 21 March 2008. 2007, [http://www.wpro.who.int/NR/rdonlyres/9AF0577E-8C21-46E2-8A46-B86191B80975/0/GFATMRDTpurchaseadvice5.pdf]Google Scholar
  18. Barnadas C, Ratsimbasoa A, Ranaivosoa H, Ralaizandry D, Raveloariseheno D, Rabekotonorina V, Picot S, Menard D: Short report: prevalence and chloroquine sensitivity of Plasmodium malariae in Madagascar. Am J Trop Med Hyg. 2007, 77: 1039-1042.PubMedGoogle Scholar
  19. Barnadas C, Tichit M, Bouchier C, Ratsimbasoa A, Randrianasolo L, Raherinjafy R, Jahevitra M, Picot S, Menard D:Plasmodium vivax dhfr and dhps mutations in isolates from Madagascar and therapeutic response to sulphadoxine-pyrimethamine. Malar J. 2008, 7: 35-10.1186/1475-2875-7-35.PubMed CentralView ArticlePubMedGoogle Scholar
  20. Menard D, Ratsimbasoa A, Randrianarivelojosia M, Rabarijaona LP, Raharimalala L, Domarle O, Randrianasolo L, Randriamanantena A, Jahevitra M, Andriantsoanirina V, Rason MA, Raherinjafy R, Rakotomalala E, Tuseo L, Raveloson A: Assessment of the efficacy of antimalarial drugs recommended by the National Malaria Control Programme in Madagascar: up-dated baseline data from randomized and multi-site clinical trials. Malar J. 2008, 7: 55-10.1186/1475-2875-7-55.PubMed CentralView ArticlePubMedGoogle Scholar
  21. Goodman SM, Benstead PB: The Natural History of Madagascar. 2003, The University of Chicago Press, Chicago and LondonGoogle Scholar
  22. Rakotonirina H, Barnadas C, Raherijafy R, Andrianantenaina H, Ratsimbasoa A, Randrianasolo L, Jahevitra M, Andriantsoanirina V, Menard D: Accuracy and reliability of malaria diagnostic techniques for guiding febrile outpatient treatment in malaria-endemic countries. Am J Trop Med Hyg. 2008, 78: 217-221.PubMedGoogle Scholar
  23. Chiodini PL, Bowers K, Jorgensen P, Barnwell JW, Grady KK, Luchavez J, Moody AH, Cenizal A, Bell D: The heat stability of Plasmodium lactate dehydrogenase-based and histidine-rich protein 2-based malaria rapid diagnostic tests. Trans R Soc Trop Med Hyg. 2007, 101: 331-337. 10.1016/j.trstmh.2006.09.007.View ArticlePubMedGoogle Scholar

Copyright

© Mariette et al; licensee BioMed Central Ltd. 2008

This article is published under license to BioMed Central Ltd. This is an Open Access article distributed under the terms of the Creative Commons Attribution License (http://creativecommons.org/licenses/by/2.0), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

Comments

By submitting a comment you agree to abide by our Terms and Community Guidelines. If you find something abusive or that does not comply with our terms or guidelines please flag it as inappropriate.

Advertisement