Skip to content

Advertisement

  • Research
  • Open Access

An innovative diagnostic technology for the codon mutation C580Y in kelch13 of Plasmodium falciparum with MinION nanopore sequencer

  • 1, 2,
  • 1, 2,
  • 3,
  • 1, 2,
  • 4,
  • 4, 5, 6, 7,
  • 8,
  • 9,
  • 10,
  • 2, 11,
  • 1, 2,
  • 3,
  • 4, 12 and
  • 2, 11Email authorView ORCID ID profile
Malaria Journal201817:217

https://doi.org/10.1186/s12936-018-2362-x

  • Received: 7 October 2017
  • Accepted: 22 May 2018
  • Published:

Abstract

Background

The recent spread of artemisinin (ART)-resistant Plasmodium falciparum represents an emerging global threat to public health. In Southeast Asia, the C580Y mutation of kelch13 (k13) is the dominant mutation of ART-resistant P. falciparum. Therefore, a simple method for the detection of C580Y mutation is urgently needed to enable widespread routine surveillance in the field. The aim of this study is to develop a new diagnostic procedure for the C580Y mutation using loop-mediated isothermal amplification (LAMP) combined with the MinION nanopore sequencer.

Results

A LAMP assay for the k13 gene of P. falciparum to detect the C580Y mutation was successfully developed. The detection limit of this procedure was 10 copies of the reference plasmid harboring the k13 gene within 60 min. Thereafter, amplicon sequencing of the LAMP products using the MinION nanopore sequencer was performed to clarify the nucleotide sequences of the gene. The C580Y mutation was identified based on the sequence data collected from MinION reads 30 min after the start of sequencing. Further, clinical evaluation of the LAMP assay in 34 human blood samples collected from patients with P. falciparum malaria in Indonesia revealed a positive detection rate of 100%. All LAMP amplicons of up to 12 specimens were simultaneously sequenced using MinION. The results of sequencing were consistent with those of the conventional PCR and Sanger sequencing protocol. All procedures from DNA extraction to variant calling were completed within 3 h. The C580Y mutation was not found among these 34 P. falciparum isolates in Indonesia.

Conclusions

An innovative method combining LAMP and MinION will enable simple, rapid, and high-sensitivity detection of the C580Y mutation of P. falciparum, even in resource-limited situations in developing countries.

Keywords

  • Malaria
  • Plasmodium falciparum
  • Artemisinin resistance
  • LAMP
  • Nanopore sequencer
  • MinION™
  • kelch 13

Background

Malaria is a mosquito-borne infectious disease and one of the most severe and prevalent public health problems in tropical and subtropical areas worldwide. In recent years, the spread of artemisinin (ART)-resistant Plasmodium falciparum malaria, which is defined as delayed parasite clearance from the blood following appropriate treatment with ART monotherapy or ART-based combination therapy (ACT) [1], has gained global attention, particularly in Southeast Asia and southern China [24]. The World Health Organization (WHO) currently recommends ACT instead of artesunate monotherapy as the first-line treatment for suspected P. falciparum malaria infections, and has urgently proposed a global plan for the monitoring and surveillance of ART-resistant P. falciparum to assess the threat of emerging resistant strains [5].

A molecular marker of ART resistance in P. falciparum has not been completely identified or validated; however, mutations in the kelch13 (k13)-propeller gene are thought to be associated with ART resistance based on in vitro and in vivo investigations [1]. Although amino acids substitutions N458Y, Y493H, R539T, I543T, R561H, and C580Y could all be associated with ART-resistance and reduce the cure rate following ACT treatment, C580Y is thought to be the dominant mutation and a potential drug resistance marker, especially in Southeast Asia [69]. Recently, ART-resistant strains of P. falciparum with C580Y mutation have spread across Cambodia, northeastern Thailand, and southern Laos. Simultaneously, the mutation could have developed resistance to piperaquine—one of the ACT partner drugs—because this drug is related to high rates of failure in the treatment of malaria [8]. Thus, there is an urgent need to strengthen the surveillance and elimination of ART-resistant P. falciparum C580Y mutation in Southeast Asia.

Point mutations and their prevalence can be confirmed by polymerase chain reaction (PCR) amplification and Sanger sequencing, which are widely used and well established. However, these techniques are unsuitable in malaria-endemic areas due to their high cost and need for sophisticated laboratories, and they cannot keep up with the current demand for field-based assays. Clinical samples need to be stored by appropriate protocols and transferred to laboratories from remote locations, which creates several disadvantages, including the cost of transportation, transfer time, and potential loss of clinical samples. Therefore, a simple and easy-to-perform molecular genotyping method is urgently required to accurately assess the distribution of ART-resistant P. falciparum in malaria-endemic areas.

Loop-mediated isothermal amplification (LAMP) is an isothermal nucleic acid amplification technique that has some operational advantages over conventional PCR procedures because it is fast, easy to use, and cost-effective [10]. Amplification is mediated by a loop structure and relies on an auto-cycling procedure performed with strand-displacement of Bst DNA polymerase under isothermal conditions. Furthermore, the amplification products in LAMP reactions can be directly judged by turbidity or changes in fluorescence with the naked eye. Given these properties, the LAMP method is expected to become an important and widely-used clinical diagnostic technique in point-of-care testing for infectious diseases and will require only limited equipment and labor. The advantages of LAMP are particularly relevant in areas with limited resources [11, 12]. Recently, Loopamp™ MALARIA Pan/Pf Detection Kit (Eiken Chemical Co., Ltd., Tokyo, Japan) has become commercially available for the detection of Plasmodium parasites.

The MinION nanopore sequencer is a pocket-sized and USB-connected portable real-time sequencer developed by Oxford Nanopore Technologies (ONT; Oxford, UK). The advantages of MinION include the simple and rapid preparation of samples, portability, real-time sequencing, relatively low cost, and the need for minimal equipment and personnel. Recently, MinION has been shown to be an alternative method for whole genome sequencing that can be used for genomic surveillance and infection control in hospitals by enabling the rapid identification of pathogens, including Ebola virus, in areas with limited resources [13, 14]. In addition, an innovative diagnostic technology using the LAMP assay combined with MinION, which is rapid, simple, highly sensitive, and cost-effective, has been introduced for the serotyping of dengue virus and genotyping of Plasmodium parasites [15, 16].

In this study, a single nucleotide polymorphism genotyping method for C580Y in k13 of P. falciparum with clinical specimens using the LAMP assay combined with MinION nanopore sequencing was developed. This is a quick, sensitive, and simple method that requires minimal equipment and personnel.

Methods

Design of LAMP primers

The oligonucleotide LAMP primers for the detection of the codon mutation of C580Y were designed based on the sequences of k13 to encompass C580Y within the F1–B1 primer pairs via online LAMP primer design software (PrimerExplorer 5, http://primerexplorer.jp/index.html; Eiken Chemical). Based on in silico analysis of the k13 sequence in six human Plasmodium parasites (P. falciparum, Plasmodium vivax, Plasmodium ovale curtisi, Plasmodium ovale wallikeri, Plasmodium knowlesi, and Plasmodium malariae), these primers were located on diverse sequences for species-specific LAMP amplification (Additional file 1: Fig. S1). The sequences of each selected primer are given in Table 1 and their positions are shown in Fig. 1.
Table 1

Nucleotide sequences of the LAMP primers constructed for kelch13 of Plasmodium falciparum

Primer

Sequence (5′–3′)

Length

LAMP primers

 F3

TGGGGGATATGATGGCTC

18

 B3

ATTATCAATACCTCCAACAACAT

23

 FIP

AGCTGATGATCTAGGGGTATTCAA-TTCTATTATACCGAATGTAGAAGCA

49

 BIP

AATGGGAACAATTTCCATATGCCT-GATTAAGGTAATTAAAAGCTGCTC

48

 LF

CCCATGCTTTCATACGATGATCATA

25

F3 and B3, outer primers; FIP and BIP, inner primers; LF, loop primer

The FIP primer consisted of F2 and the complementary strand (F1c)

The BIP primer consisted of B2 and the complementary strand (B1c)

Fig. 1
Fig. 1

Alignment of the partial sequences of the kelch13 of Plasmodium falciparum, which was constructed within the pEX-A2J1 plasmid. The constructed sets of LAMP primers are shown as lines and boxes. Asterisks show the specific sequences located at the codon position of C580Y in artemisinin-resistant P. falciparum

Plasmid construction

The templates used for the analytical LAMP reactions were the pEX-A2J1 plasmids harbouring partial sequences within the k13 of P. falciparum, which were constructed by Eurofines Genomics Co., Ltd. (Tokyo, Japan) based on the reference sequences (GenBank accession numbers: P. falciparum, KT956001.1 and KR537460.1). The sequences of the constructed plasmids are summarized in Fig. 1. The plasmids were serially diluted tenfold and adjusted from 1.0 × 101 to 1.0 × 105 copies/μL to determine the detection threshold and specificity of the LAMP reactions. The sequences of the constructed plasmids were confirmed by the Sanger method using F3 and B3 primers (Table 1).

LAMP reactions

The reactions were performed using a Loopamp DNA Amplification Reagent Kit (Eiken Chemical). Detection of the LAMP amplicons was performed by real-time measurements of turbidity using a Loopamp real-time turbidimeter LA-200 (Eiken Chemical) and visual observations of the colour changes with the naked eye under natural light. The final reaction volume was 25 μL, comprising 40 pmol of the FIP primer and 40 pmol of the BIP primer, 20 pmol of each loop primer, 5 pmol of F3 and B3 primers, 1 μL of the Bst DNA polymerase, reaction buffer (20 mM Tris–HCl, 10 mM KCl, 8 mM MgSO4, 10 mM (NH4)2SO4, 0.1% Tween 20, 0.8 M betaine, and 1.4 mM each dNTP), and 1 μL of plasmid DNA or 8 μL of genomic DNA samples. Reactions were carried out at 62, 63, 64, and 65 °C in duplicate to find the optimum temperature for the LAMP amplification.

The detection limit and specificity of the LAMP assay

Ten-fold serial dilutions of each plasmid DNA ranging from 1.0 × 101 to 1.0 × 105 copies/μL were produced to determine the detection limit of the LAMP primers, and stored at − 20 °C in duplicate until use. Additionally, to evaluate the specificity of the test, seven different protozoa (Toxoplasma gondii, Cryptosporidium parvum, Giardia intestinalis, Entamoeba histolytica, Leishmania donovani, Trypanosoma brucei rhodesiense, and Trypanosoma cruzi) isolated by the National BioResource Project (http://www.nbrp.jp/) were also examined.

Clinical samples and ethics

Clinical samples were obtained from Sam Ratulangi University in Manado and Bitung, North Sulawesi, Indonesia from August to December 2010. All patients were diagnosed based on symptoms, blood smears stained with Giemsa stain, and nested PCR according to previously reported protocols [1719]. Peripheral blood was collected by FTA Elute cards (GE Healthcare Life Sciences, Little Chalfont, UK) from each patient and stored at room temperature.

Both the design and protocol of this study conformed to the Helsinki Declaration and were approved by the Institutional Ethics Committee. All samples were collected after written informed consent has been obtained. The methods of collection and analysis of the human samples were approved and cleared by the Institutional Ethical Review Board of Sam Ratulangi University and the University of Tokyo.

DNA extraction from clinical samples

Genomic DNA was extracted following the manufacturer’s instructions for FTA Elute cards. Briefly, each disk with a diameter of 3.0 mm was cut from the blood spot areas and washed three times with 200 μL of distilled water. DNA was eluted in 30 μL of TE buffer (10 mM Tris–HCl, 0.1 mM EDTA, pH 8.0) with a heat block at 95 °C for 30 min. Finally, 8.0 μL of supernatant was used as template DNA for both LAMP assays.

Sequencing of LAMP products by MinION

To confirm the presence of codon mutation C580Y in k13, amplicon sequencing of LAMP reactions by MinION sequencer was performed. LAMP amplicons derived from plasmid DNA harboring partial sequences of k13 with or without C580Y mutation and clinical samples were purified with Agencourt AMPure XP beads (Beckman Coulter Inc., Brea, CA). For the multiplex and real-time MinION sequencing, a Rapid Barcoding Sequencing Kit (SQK-RBK001, ONT) was used to sequence up to 12 samples on a single flow cell. LAMP amplicons (200 ng each) were measured by Qubit 3.0 Fluorometer (Thermo Fisher Scientific) and simultaneously processed for the barcoding and library preparation using the Rapid Barcoding Sequencing Kit, according to the manufacturer’s instructions. After the MinION Platform QC run, the DNA library was loaded into MinION Flow Cell (FLO-MIN107 R9.5 Version) and the “NC_48Hr_sequencing_FLO-MIN107_SQK-RBK001_plus_basecaller” protocol was initiated using MinKNOW software (ONT, v1.4.2).

Analysis of MinION data

Figure 2 shows the workflow of the data analysis in this study. Local basecalling was performed using MinKNOW in real time and automatically. FAST5 reads were collected at 30 min and 48 h after the start of sequencing. FASTQ files were extracted from each collected FAST5 read via Poretools (v 0.6.0). Demultiplexing and adapter trimming was performed using Porechop (v 0.2.2), and each FASTQ per ONT-barcode data was mapped by BWA-MEM (v 0.7.15) using the sequence of k13 without the C580Y codon mutation between a pair of LAMP primers, F1c (5′-TTG AAT ACC CCT AGA TCA TCA GC-3′) and B1c (5′-AAT GGG AAC AAT TTC CAT ATG CCT-3′). The mapped data with a “MapQuality” < 60 were discarded via Samtools (v 1.5.0). The single nucleotide variant calling from mapped data was obtained via Samtools and BCFtools (v 1.5.0), and cutoff values of 50 for single nucleotide variant quality and read depth were determined. Mapped data were visualized by IGV software (v 2.3.8). FAST5 reads and mapped data were analysed via Poretools and Samtools, respectively.
Fig. 2
Fig. 2

Schematic of the data analysis workflow in this study

k13 amplification and Sanger sequencing

The Sanger method was used to perform PCR amplicon sequencing to confirm and validate the sequence results of LAMP amplicons via the MinION sequencer for the clinical specimens. For the specific amplification of k13, nested PCR according to previously reported protocols were used [7]. Briefly, the first- and second-round PCR amplicons were generated by PrimeSTAR GXL DNA Polymerase (Takara Bio Inc., Kusatsu, Japan) with the following primers: first round forward primers, 5′-CGG AGT GAC CAA ATC TGG GA-3′ and reverse primers, 5′-GGG AAT CTG GTG GTA ACA GC-3′; second round forward primers, 5′-GCC AAG CTG CCA TTC ATT TG-3′ and reverse primers, 5′-GCC TTG TTG AAA GAA GCA GA-3′. Thermal cycling was carried out under the following conditions: 94 °C for 2 min, followed by 40 cycles at 98 °C for 10 s, 55 °C for 30 s, 68 °C for 1 min, with a final extension at 68 °C for 7 min in both the first- and second-round amplifications. The 1000-fold dilution products of the first round of PCR were used as templates for the second round. All second-round PCR products were analyzed using 1.2% (w/v) agarose gel, stained with ethidium bromide, and purified by Agencourt AMPure XP beads (Beckman Coulter). Sanger sequencing of these purified PCR amplicons was performed by Eurofines Genomics Co., Ltd. (Tokyo, Japan).

Results

Sensitivity and specificity of LAMP

A tenfold serial dilution of each plasmid DNA was amplified to determine the lower detection limit of the constructed LAMP assay and the optimal temperature was observed at 62 °C. Figure 3 shows the results of detection based on real-time turbidity; amplification of the target DNA is indicated by the rising curve. The minimum amounts of plasmid DNA on real-time turbidities with LA-200 were 1.0 × 101/reaction within 60 min (Fig. 2). These results were similar to those obtained by observing visual changes within 60 min. Additionally, 1.0 ng of genomic DNA derived from seven other protozoa (Toxoplasma gondii, Cryptosporidium parvum, Giardia intestinalis, Entamoeba histolytica, Leishmania donovani, Trypanosoma brucei rhodesiense, and Trypanosoma cruzi) were not amplified by the LAMP procedure.
Fig. 3
Fig. 3

The detection limit of LAMP for kelch13 of Plasmodium falciparum with tenfold serial dilutions of plasmid DNA

Clinical evaluation of LAMP assays

Parasitemia was confirmed in 40 blood samples by nested-PCR (33 P. falciparum, 6 P. vivax, and 1 co-infection with P. falciparum and P. vivax). All 33 P. falciparum and the 1 co-infection cases were positive (n = 34; 100%). None of the 6 P. vivax blood samples were amplified with the LAMP primers (Table 2).
Table 2

Summary of the results of nested PCR and LAMP amplifications, and the identification of kelch13 mutations of P. falciparum

 

LAMP reaction

Identification of mutation

PCR and Sanger

LAMP and MinION

Positive

Negative

C580Y

Wild type

C580Y

Wild type

Nested PCR

 P. f

33

33

0

0

33

0

33

 P. f/P. v

1

1

0

0

1

0

1

 P. v

6

0

6

P. f, P. falciparum; P. v, P. vivax; P.f/P.v, P. falciparum and P. vivax co-infection

Sequencing of LAMP products by MinION

Figure 4 and Additional file 2: Table S1 show the results of FAST5 reads analysis generated 30 min after the start of MinION sequencing. The mean collected read numbers and read bases per run were 10,052 and 2215, respectively. Of the total collected reads, 1.57–7.75% were classified into ONT-barcodes after barcode demultiplexing; however, reads from 35.8 to 70.6% were unclassified. Based on the analysis of the mapped data, a depth of coverage above 50× was achieved at each base on the reference sequence. Because LAMP amplicons contain random repeating structures, a read was mapped as a reference sequence more than once by BWA-MEM.
Fig. 4
Fig. 4

The results of FAST5 reads analysis collected 30 min from the start of MinION sequencing. a Histogram of FAST5 read sizes from each MinION sequencing run. b Collector’s curve reflecting the total base pairs of sequencing yield over time for each MinION sequencing run. c Depth of coverage for each ONT-barcode number and MinION sequencing run

Table 3 showed the results of mapped data obtained from the analysis workflow using LAMP amplicons with plasmids harbouring the partial sequences of k13 with or without the C580Y mutation. Variant callings from collected reads were consistent with the plasmid sequences. The average accuracy of the mapped reads of LAMP amplicons generated from plasmids with the codon mutation C580Y was 89.0%, and at the base of the mutation C580Y (position 6/from “G” to “A”), 86.4% reads were correctly matched with “A”, but 13.6% reads were mismatched (Additional file 3: Fig. S2, Additional file 2: Table S2).
Table 3

Summary of the MinION sequencing of LAMP amplicons from plasmids

Reference plasmid

Total reads

Mapped reads > MQ60

Coverage

% bases depth > 50

Accuracy (%)

Sequencing result

C580Y

389

793

748.10

100

89.54

C580Y

Wild type

476

822

761.83

100

89.9

Wild type

None of the 34 LAMP amplicons from clinical specimens showed the C580Y mutation based on variant calling from collected reads at 30 min. These results were consistent with the results of PCR amplicon sequencing by conventional Sanger methods (Table 2 and Additional file 2: Table S1). In addition, the same analysis of reads collected 48 h after the start of MinION sequencing were also performed (Additional file 4: Fig. S3 and Additional file 2: Table S3). The results of variant calling were consistent with the results at 30 min.

Discussion

Although several sophisticated LAMP methods have been developed for the detection of Plasmodium parasites from clinical specimens [11, 12, 2033], none have been designed to detect single nucleotide polymorphisms (SNPs) associated with ART resistance in P. falciparum. The LAMP method combined with MinION sequencing method was capable of simultaneously detecting both P. falciparum parasitaemia and the codon mutation in k13 in up to 12 samples at a high level of sensitivity without expensive or large experimental devices. The practical advantage of this method is that it enables real-time monitoring of ART resistance in patients diagnosed with P. falciparum malaria, even in areas with limited resources, because the samples can be prepared and sequenced without storage or transfer to a fully-equipped laboratory. Another advantage of this protocol is that sequence data can be stored in the cloud and shared at anytime, anywhere in the world.

The gold standard diagnostic method for malaria to date is the microscopic examination of Giemsa-stained thin or thick blood smears. Several rapid diagnostic tests (RDT), such as the rapid immunochromatographic test, are already manufactured and used throughout the world. However, misdiagnosis is common in microscopic examinations or rapid immunochromatographic tests of mixed infections when a patient has low-density parasitemia or is asymptomatic [3436]. Consequently, low-density parasitaemia or asymptomatic carriers of P. falciparum could be reservoirs for malaria infections [37, 38]. Therefore, highly sensitive diagnostic tools that can detect even low-density parasitaemia are essential for the elimination and accurate epidemiological surveillance of ART-resistant P. falciparum. Molecular diagnostic tests such as PCR or LAMP methods are highly sensitive and can detect plasmodium infections even at very low levels of parasitaemia [20, 3942]. In particular, the detection limit of standard nested-PCR [18], real-time PCR [43], and commercial LAMP assay for malaria (Loopamp™ MALARIA Pan/Pf Detection Kit, Eiken Chemical, Japan) are respectively 6.0, 0.7, and 25.0 parasites/mL, and exceed the detection limit of both microscopy (50–500 parasites/mL) [44, 45] and RDT for P. falciparum-specific histidine-rich protein II, Plasmodium lactate dehydrogenase, or aldolase (100 parasites/mL) [44]. In this study, the detection limit of the LAMP method for k13 gene was 1.0 × 10 copies/reaction (corresponding to 12.5 parasite/mL), and the levels of sensitivity and specificity were 100% in the clinical samples. The sensitivity of the LAMP assay is equivalent to previously described LAMP assays (sensitivity ~ 100% and specificity ~ 100%) [11, 12, 2033].

Using the high specificity of the LAMP method, techniques for genotyping gene polymorphisms without sequence analysis have been developed, including LAMP with FIP and/or BIP primers, which are designed to contain a single-nucleotide polymorphism at each 5′ end (SNPs-LAMP) (http://loopamp.eiken.co.jp/) or insert artificial mutations using FIP and/or BIP primers (ARMS-LAMP) [46, 47]. However, the design of LAMP primers for the above-mentioned protocol is not only quite difficult and limited, but also less sensitive than conventional LAMP assays [48]. In contrast, the LAMP method combined with MinION sequencing can achieve unlimited LAMP primer designs for genotyping polymorphisms.

A diagnostic method for dengue virus via the real-time LAMP method combined with MinION sequencer has been previously developed [16]. However, the multiplex sequence methods for that protocol use barcoded-LAMP FIP primers, which insert a unique 24-base ONT-barcode tag within the F1c sites. In this study, the detection limit of “Barcode-LAMP FIP primers” was one-hundredth that of the “Non-barcoded LAMP FIP primers” (1.0 × 103 copies/reaction vs 1.0 × 10 copies/reaction), and the “Barcode-LAMP FIP primers” can detect only 85.7% of P. falciparum parasitaemia cases (Additional file 5: Fig. S4, Additional file 2: Tables S4, S5). In the study by Yamagishi et al., the sensitivity of real-time LAMP in the clinical cases was only 80%, and the LAMP reaction took 90 min. The sensitivity of the above-mentioned LAMP assay was inferior to previously reported LAMP assays for dengue virus (sensitivity ~ 100%) [4951]. In addition, the protocol took over 2 h to prepare the library using the Ligation Sequencing Kit (SQK-LSK002). In this study, all procedures from DNA extraction to variant calling were completed within 3 h.

It is well documented that MinION reads have a much higher error rate, especially via 1D-chemistry, than conventional Sanger sequencing or other next generation sequencing platforms, including 454, Illumina, and Iontorrent technology [5255]. The rate of accuracy of 1D-read chemistry with R9.4 flow cell is about 90% (https://nanoporetech.com/). To generate accurate sequences, genomic regions must be read multiple times, with errors eliminated through consensus averaging. Because of the high error rate of MinION, a 50-fold read coverage of the genome positions was sufficient to accurately determine the genotypes. LAMP amplicons are constructed of complicated repeating structures; therefore, a single read generated from MinION contains several multiple base sequences of the target region. This LAMP method combined with MinION sequencing could collect sufficient sequence data within 30 min of starting MinION sequencing. The results of variant calling by this method were completely consistent with the results of Sanger sequencing. Therefore, this procedure is a highly accurate method of variant calling. However, it did not achieve sufficient accuracy for deep sequencing to detect low-frequency mutations within a sample because the average rate of accuracy was 89.4%.

Therefore, if the proportion of the C580Y mutant strain is smaller than that of the wild type strain in the same clinical specimen, the C580Y mutation may not be accurately detected. It is thought that this disparity occurred for the following reasons: the high error rate of MinION reads, the fidelity of the LAMP enzyme, and the mapping algorithm of BWA-MEM. ONT has introduced 1D2-read chemistry with higher precision than 1D-read chemistry (https://nanoporetech.com/), which will improve the precision of the combined LAMP and MinION sequencer method in the future.

This study was limited due to the small number of malaria samples; hence, the performance of the sensitivity and specificity in clinical samples have not been demonstrated. The specificity in clinical samples that contained only P. vivax were evaluated. In addition, there were no C580Y mutations in k13 found among 34 P. falciparum isolates collected in 2010 in Indonesia. An accurate evaluation of the sensitivity and specificity of this method requires further investigation in a clinical setting.

The LAMP method combined with MinION sequencing detected SNPs only in the 95 bp region incorporating the C580Y codon mutation in k13 amplified by the LAMP primers. The other codon mutations in k13 are reportedly associated with ART resistance. This procedure will be used to detect other mutations for the surveillance of ART resistance in the next study. Due to the flexibility afforded in the design of LAMP primers, this procedure can easily be used to detect other SNPs associated with drug-resistance genes not only in P. falciparum, but also in bacteria or fungi.

Conclusions

In this study, an innovative diagnostic technology to detect the codon mutation C580Y in k13 of P. falciparum was demonstrated. The method, which uses the LAMP assay combined with MinION sequencer, is rapid, simple, and highly sensitive. This procedure could contribute to the epidemiological surveillance of ART-resistant P. falciparum and be applied to the analyses of sequence polymorphisms or genotyping. The next step for refining this procedure will be to conduct a clinical evaluation to verify that the sensitivity and specificity are sufficient and consistent in resource-limited endemic regions.

Declarations

Authors’ contributions

JT, YS, JY, and TMa conceived and designed the study; KI, NT, LRR, JS, and TMa gathered and analysed the data, and drafted and edited the manuscript; KH, YE, RM, HO, TMu, SM, YS, and JY supervised the study and revised the manuscript; YS, JY, and TMa performed project administration. All authors read and approved the final manuscript.

Acknowledgements

This work was supported in part by the National BioResource Project in Japan. (http://www.nbrp.jp/).

Competing interests

The authors declare that they have no competing interests.

Availability of data and materials

The datasets supporting the conclusions of this article are included within the article.

Consent for publication

Not applicable.

Ethics approval and consent to participate

Ethical clearances were obtained from Institutional Ethical Review Board of Sam Ratulangi University and The University of Tokyo (Approval Number 10-49). The purpose of the study was explained in detail and written, informed consent was obtained from all participants. Confidentiality was maintained by avoiding the use of names and other identifiers.

Funding

This research did not receive any specific grant from funding agencies in the public, commercial, or not-for-profit sectors.

Publisher’s Note

Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Open AccessThis article is distributed under the terms of the Creative Commons Attribution 4.0 International License (http://creativecommons.org/licenses/by/4.0/), which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated.

Authors’ Affiliations

(1)
Department of Infectious Disease and Infection Control, Saitama Medical University, 38 Morohongo, Moroyama-machi, Iruma-gun Saitama, 350-0495, Japan
(2)
Center for Clinical Infectious Diseases and Research, Saitama Medical University, 38 Morohongo, Moroyama-machi, Iruma-gun Saitama, 350-0495, Japan
(3)
Department of Computational Biology and Medical Science, Graduate School of Frontier Sciences, The University of Tokyo, 5-1-5 Kashiwanoha, Kashiwa Chiba, 277-8562, Japan
(4)
Research Center for Zoonosis Control, Hokkaido University, North 20, West 10 Kita-ku, Sapporo Hokkaido, 001-0020, Japan
(5)
Faculty of Medicine, Oita University, 1-1 Hasama-machi, Yufu Oita, 879-5593, Japan
(6)
Department of Medical Entomology, Faculty of Tropical Medicine, Mahidol University, 420/6 Ratchawithi Road, Thung Phaya, Ratchathewi, Bangkok, 10400, Thailand
(7)
Research Institute for Microbial Diseases, Osaka University, 3-1 Yamadaoka, Suita Osaka, 565-0871, Japan
(8)
Division of Biomedical Sciences, Department of Basic Veterinary Medicine, Obihiro University of Agriculture and Veterinary Medicine, 2-11 Inada-cho, Obihiro Hokkaido, 080-8555, Japan
(9)
Department of Parasitology, Faculty of Medicine, Sam Ratulangi University, Kampus Unsrat, Bahu Manado, 95115, Indonesia
(10)
Department of Infectious Diseases and Infection Control, Saitama Medical Center, Saitama Medical University, 1981 Kamoda, Kawagoe Saitama, 350-8550, Japan
(11)
Department of Microbiology, Saitama Medical University, 38 Morohongo, Moroyama-machi, Iruma-gun Saitama, 350-0495, Japan
(12)
Global Station for Zoonosis Control, GI-CoRE, Hokkaido University, North 20, West 10 Kita-ku, Sapporo Hokkaido, 001-0020, Japan

References

  1. WHO. Global Malaria Programme Artemisinin and artemisinin-based combination therapy resistance. Status report. Geneva: World Health Organization; 2016.Google Scholar
  2. Dondorp AM, Nosten F, Yi P, Das D, Phyo AP, Tarning J, et al. Artemisinin resistance in Plasmodium falciparum malaria. N Engl J Med. 2009;361:455–67.View ArticlePubMedPubMed CentralGoogle Scholar
  3. Hawkes M, Conroy AL, Kain KC. Spread of artemisinin resistance in malaria. N Engl J Med. 2014;371:1944–5.View ArticlePubMedGoogle Scholar
  4. Noedl H, Se Y, Schaecher K, Smith BL, Socheat D, Fukuda MM. Evidence of artemisinin-resistant malaria in western Cambodia. N Engl J Med. 2008;359:2619–20.View ArticlePubMedGoogle Scholar
  5. WHO. Guidelines for the treatment of malaria. 3rd ed. Geneva: World Health Organization; 2015.Google Scholar
  6. Miotto O, Amato R, Ashley EA, MacInnis B, Almagro-Garcia J, Amaratunga C, et al. Genetic architecture of artemisinin-resistant Plasmodium falciparum. Nat Genet. 2015;47:226–34.View ArticlePubMedPubMed CentralGoogle Scholar
  7. Ariey F, Witkowski B, Amaratunga C, Beghain J, Langlois AC, Khim N, et al. A molecular marker of artemisinin-resistant Plasmodium falciparum malaria. Nature. 2014;505:50–5.View ArticlePubMedGoogle Scholar
  8. Imwong M, Suwannasin K, Kunasol C, Sutawong K, Mayxay M, Rekol H, et al. The spread of artemisinin-resistant Plasmodium falciparum in the Greater Mekong subregion: a molecular epidemiology observational study. Lancet Infect Dis. 2017;17:491–7.View ArticlePubMedPubMed CentralGoogle Scholar
  9. Imwong M, Jindakhad T, Kunasol C, Sutawong K, Vejakama P, Dondorp AM. An outbreak of artemisinin resistant falciparum malaria in Eastern Thailand. Sci Rep. 2015;5:17412.View ArticlePubMedPubMed CentralGoogle Scholar
  10. Mori Y, Notomi T. Loop-mediated isothermal amplification (LAMP): a rapid, accurate, and cost-effective diagnostic method for infectious diseases. J Infect Chemother. 2009;15:62–9.View ArticlePubMedGoogle Scholar
  11. Morris U, Khamis M, Aydin-Schmidt B, Abass AK, Msellem MI, Nassor MH, et al. Field deployment of loop-mediated isothermal amplification for centralized mass-screening of asymptomatic malaria in Zanzibar: a pre-elimination setting. Malar J. 2015;14:205.View ArticlePubMedPubMed CentralGoogle Scholar
  12. Aydin-Schmidt B, Xu W, Gonzalez IJ, Polley SD, Bell D, Shakely D, et al. Loop mediated isothermal amplification (LAMP) accurately detects malaria DNA from filter paper blood samples of low density parasitaemias. PLoS One. 2014;9:e103905.View ArticlePubMedPubMed CentralGoogle Scholar
  13. Quick J, Ashton P, Calus S, Chatt C, Gossain S, Hawker J, et al. Rapid draft sequencing and real-time nanopore sequencing in a hospital outbreak of Salmonella. Genome Biol. 2015;16:114.View ArticlePubMedPubMed CentralGoogle Scholar
  14. Kugelman JR, Wiley MR, Mate S, Ladner JT, Beitzel B, Fakoli L, et al. Monitoring of Ebola Virus Makona evolution through establishment of advanced genomic capability in Liberia. Emerg Infect Dis. 2015;21:1135–43.View ArticlePubMedPubMed CentralGoogle Scholar
  15. Elia MIY, Isra W, Mochammad H. The evaluation on molecular techniques of reverse transcription loop-mediated isothermal amplification (RT-LAMP), reverse transcription polymerase chain reaction (RT-PCR), and their diagnostic results on MinION™ Nanopore sequencer for the detection of dengue virus serotypes. Am J Microbiol Res. 2015;3:118–24.Google Scholar
  16. Yamagishi J, Runtuwene LR, Hayashida K, Mongan AE, Thi LAN, Thuy LN, et al. Serotyping dengue virus with isothermal amplification and a portable sequencer. Sci Rep. 2017;7:3510.View ArticlePubMedPubMed CentralGoogle Scholar
  17. Iwasaki M, Toshihiro Y, Otsuka K, Suzuki W, Nagamine K, Hase T, et al. Validation of the loop-mediated isothermal amplification method for single nucleotide polymorphism genotyping with whole blood. Genome Lett. 2003;2:119–26.View ArticleGoogle Scholar
  18. Singh B, Bobogare A, Cox-Singh J, Snounou G, Abdullah MS, Rahman HA. A genus- and species-specific nested polymerase chain reaction malaria detection assay for epidemiologic studies. Am J Trop Med Hyg. 1999;60:687–92.View ArticlePubMedGoogle Scholar
  19. Singh B, Kim Sung L, Matusop A, Radhakrishnan A, Shamsul SS, Cox-Singh J, et al. A large focus of naturally acquired Plasmodium knowlesi infections in human beings. Lancet. 2004;363:1017–24.View ArticlePubMedGoogle Scholar
  20. Cook J, Aydin-Schmidt B, Gonzalez IJ, Bell D, Edlund E, Nassor MH, et al. Loop-mediated isothermal amplification (LAMP) for point-of-care detection of asymptomatic low-density malaria parasite carriers in Zanzibar. Malar J. 2015;14:43.View ArticlePubMedPubMed CentralGoogle Scholar
  21. Cuadros J, Perez-Tanoira R, Prieto-Perez L, Martin-Martin I, Berzosa P, Gonzalez V, et al. Field evaluation of malaria microscopy, rapid malaria tests and loop-mediated isothermal amplification in a rural hospital in South Western Ethiopia. PLoS One. 2015;10:e0142842.View ArticlePubMedPubMed CentralGoogle Scholar
  22. Hayashida K, Simukoko H, Simmunza M, Ndebe J, Chota A, Namangala B, et al. Direct detection of falciparum and non-falciparum malaria DNA from a drop of blood with high sensitivity by the dried-LAMP system. Parasit Vectors. 2017;10:26.View ArticlePubMedPubMed CentralGoogle Scholar
  23. Hopkins H, Gonzalez IJ, Polley SD, Angutoko P, Ategeka J, Asiimwe C, et al. Highly sensitive detection of malaria parasitemia in a malaria-endemic setting: performance of a new loop-mediated isothermal amplification kit in a remote clinic in Uganda. J Infect Dis. 2013;208:645–52.View ArticlePubMedPubMed CentralGoogle Scholar
  24. Lau YL, Fong MY, Mahmud R, Chang PY, Palaeya V, Cheong FW, et al. Specific, sensitive and rapid detection of human Plasmodium knowlesi infection by loop-mediated isothermal amplification (LAMP) in blood samples. Malar J. 2011;10:197.View ArticlePubMedPubMed CentralGoogle Scholar
  25. Lau YL, Lai MY, Fong MY, Jelip J, Mahmud R. Loop-mediated isothermal amplification assay for identification of five human plasmodium species in Malaysia. Am J Trop Med Hyg. 2016;94:336–9.View ArticlePubMedPubMed CentralGoogle Scholar
  26. Lee PW, Ji DD, Liu CT, Rampao HS, do Rosario VE, Lin IF, et al. Application of loop-mediated isothermal amplification for malaria diagnosis during a follow-up study in Sao Tome. Malar J. 2012;11:408.View ArticlePubMedPubMed CentralGoogle Scholar
  27. Lucchi NW, Demas A, Narayanan J, Sumari D, Kabanywanyi A, Kachur SP, et al. Real-time fluorescence loop mediated isothermal amplification for the diagnosis of malaria. PLoS One. 2010;5:e13733.View ArticlePubMedPubMed CentralGoogle Scholar
  28. Lucchi NW, Ljolje D, Silva-Flannery L, Udhayakumar V. Use of malachite green-loop mediated isothermal amplification for detection of Plasmodium spp. parasites. PLoS One. 2016;11:e0151437.View ArticlePubMedPubMed CentralGoogle Scholar
  29. Modak SS, Barber CA, Geva E, Abrams WR, Malamud D, Ongagna YS. Rapid point-of-care isothermal amplification assay for the detection of malaria without nucleic acid purification. Infect Dis (Auckl). 2016;9:1–9.View ArticlePubMedPubMed CentralGoogle Scholar
  30. Mohon AN, Elahi R, Khan WA, Haque R, Sullivan DJ Jr, Alam MS. A new visually improved and sensitive loop mediated isothermal amplification (LAMP) for diagnosis of symptomatic falciparum malaria. Acta Trop. 2014;134:52–7.View ArticlePubMedGoogle Scholar
  31. Oriero EC, Okebe J, Jacobs J, Van Geertruyden JP, Nwakanma D, D’Alessandro U. Diagnostic performance of a novel loop-mediated isothermal amplification (LAMP) assay targeting the apicoplast genome for malaria diagnosis in a field setting in sub-Saharan Africa. Malar J. 2015;14:396.View ArticlePubMedPubMed CentralGoogle Scholar
  32. Patel JC, Lucchi NW, Srivastava P, Lin JT, Sug-Aram R, Aruncharus S, et al. Field evaluation of a real-time fluorescence loop-mediated isothermal amplification assay, RealAmp, for the diagnosis of malaria in Thailand and India. J Infect Dis. 2014;210:1180–7.View ArticlePubMedGoogle Scholar
  33. Sirichaisinthop J, Buates S, Watanabe R, Han ET, Suktawonjaroenpon W, Krasaesub S, et al. Evaluation of loop-mediated isothermal amplification (LAMP) for malaria diagnosis in a field setting. Am J Trop Med Hyg. 2011;85:594–6.View ArticlePubMedPubMed CentralGoogle Scholar
  34. Cheng Q, Cunningham J, Gatton ML. Systematic review of sub-microscopic P. vivax infections: prevalence and determining factors. PLoS Negl Trop Dis. 2015;9:e3413.View ArticlePubMedPubMed CentralGoogle Scholar
  35. Okell LC, Ghani AC, Lyons E, Drakeley CJ. Submicroscopic infection in Plasmodium falciparum-endemic populations: a systematic review and meta-analysis. J Infect Dis. 2009;200:1509–17.View ArticlePubMedGoogle Scholar
  36. Falade CO, Ajayi IO, Nsungwa-Sabiiti J, Siribie M, Diarra A, Serme L, et al. Malaria rapid diagnostic tests and malaria microscopy for guiding malaria treatment of uncomplicated fevers in Nigeria and prereferral cases in 3 African countries. Clin Infect Dis. 2016;63:S290–7.View ArticlePubMedPubMed CentralGoogle Scholar
  37. Lindblade KA, Steinhardt L, Samuels A, Kachur SP, Slutsker L. The silent threat: asymptomatic parasitemia and malaria transmission. Expert Rev Anti Infect Ther. 2013;11:623–39.View ArticlePubMedGoogle Scholar
  38. Bousema T, Drakeley C. Epidemiology and infectivity of Plasmodium falciparum and Plasmodium vivax gametocytes in relation to malaria control and elimination. Clin Microbiol Rev. 2011;24:377–410.View ArticlePubMedPubMed CentralGoogle Scholar
  39. Baltzell KA, Shakely D, Hsiang M, Kemere J, Ali AS, Bjorkman A, et al. Prevalence of PCR detectable malaria infection among febrile patients with a negative Plasmodium falciparum specific rapid diagnostic test in Zanzibar. Am J Trop Med Hyg. 2013;88:289–91.View ArticlePubMedPubMed CentralGoogle Scholar
  40. Kattenberg JH, Tahita CM, Versteeg IA, Tinto H, Traore Coulibaly M, D’Alessandro U, et al. Evaluation of antigen detection tests, microscopy, and polymerase chain reaction for diagnosis of malaria in peripheral blood in asymptomatic pregnant women in Nanoro, Burkina Faso. Am J Trop Med Hyg. 2012;87:251–6.View ArticlePubMedPubMed CentralGoogle Scholar
  41. Kyabayinze DJ, Zongo I, Cunningham J, Gatton M, Angutoko P, Ategeka J, et al. HRP2 and pLDH-based rapid diagnostic tests, expert microscopy, and PCR for detection of malaria infection during pregnancy and at delivery in areas of varied transmission: a prospective cohort study in Burkina Faso and Uganda. PLoS One. 2016;11:e0156954.View ArticlePubMedPubMed CentralGoogle Scholar
  42. Wu L, van den Hoogen LL, Slater H, Walker PG, Ghani AC, Drakeley CJ, et al. Comparison of diagnostics for the detection of asymptomatic Plasmodium falciparum infections to inform control and elimination strategies. Nature. 2015;528:S86–93.View ArticlePubMedGoogle Scholar
  43. Perandin F, Manca N, Calderaro A, Piccolo G, Galati L, Ricci L, et al. Development of a real-time PCR assay for detection of Plasmodium falciparum, Plasmodium vivax, and Plasmodium ovale for routine clinical diagnosis. J Clin Microbiol. 2004;42:1214–9.View ArticlePubMedPubMed CentralGoogle Scholar
  44. Wongsrichanalai C, Barcus MJ, Muth S, Sutamihardja A, Wernsdorfer WH. A review of malaria diagnostic tools: microscopy and rapid diagnostic test (RDT). Am J Trop Med Hyg. 2007;77:119–27.PubMedView ArticleGoogle Scholar
  45. Milne LM, Kyi MS, Chiodini PL, Warhurst DC. Accuracy of routine laboratory diagnosis of malaria in the United Kingdom. J Clin Pathol. 1994;47:740–2.View ArticlePubMedPubMed CentralGoogle Scholar
  46. Tamura S, Maeda T, Misawa K, Osa M, Hamamoto T, Yuki A, et al. Development of a highly resolved loop-mediated isothermal amplification method to detect the N526K ftsI mutation of beta-lactamase-negative ampicillin-resistant Haemophilus influenzae. J Microbiol Methods. 2017;141:108–14.View ArticlePubMedGoogle Scholar
  47. Lee D, Kim EJ, Kilgore PE, Takahashi H, Ohnishi M, Tomono J, et al. A novel loop-mediated isothermal amplification assay for serogroup identification of Neisseria meningitidis in cerebrospinal fluid. Front Microbiol. 2015;6:1548.PubMedGoogle Scholar
  48. Torigoe H, Seki M, Yamashita Y, Sugaya A, Maeno M. Detection of Haemophilus influenzae by loop-mediated isothermal amplification (LAMP) of the outer membrane protein P6 gene. Jpn J Infect Dis. 2007;60:55–8.PubMedGoogle Scholar
  49. Parida M, Horioke K, Ishida H, Dash PK, Saxena P, Jana AM, et al. Rapid detection and differentiation of dengue virus serotypes by a real-time reverse transcription-loop-mediated isothermal amplification assay. J Clin Microbiol. 2005;43:2895–903.View ArticlePubMedPubMed CentralGoogle Scholar
  50. Hu SF, Li M, Zhong LL, Lu SM, Liu ZX, Pu JY, et al. Development of reverse-transcription loop-mediated isothermal amplification assay for rapid detection and differentiation of dengue virus serotypes 1-4. BMC Microbiol. 2015;15:265.View ArticlePubMedPubMed CentralGoogle Scholar
  51. Teoh BT, Sam SS, Tan KK, Johari J, Danlami MB, Hooi PS, et al. Detection of dengue viruses using reverse transcription-loop-mediated isothermal amplification. BMC Infect Dis. 2013;13:387.View ArticlePubMedPubMed CentralGoogle Scholar
  52. Schirmer M, Ijaz UZ, D’Amore R, Hall N, Sloan WT, Quince C. Insight into biases and sequencing errors for amplicon sequencing with the Illumina MiSeq platform. Nucleic Acids Res. 2015;43:e37.View ArticlePubMedPubMed CentralGoogle Scholar
  53. Shao W, Boltz VF, Spindler JE, Kearney MF, Maldarelli F, Mellors JW, et al. Analysis of 454 sequencing error rate, error sources, and artifact recombination for detection of low-frequency drug resistance mutations in HIV-1 DNA. Retrovirology. 2013;10:18.View ArticlePubMedPubMed CentralGoogle Scholar
  54. Liu L, Li Y, Li S, Hu N, He Y, Pong R, et al. Comparison of next-generation sequencing systems. J Biomed Biotechnol. 2012;2012:251364.PubMedPubMed CentralGoogle Scholar
  55. Jain M, Tyson JR, Loose M, Ip CLC, Eccles DA, O’Grady J, et al. MinION analysis and reference consortium: phase 2 data release and analysis of R9.0 chemistry. F1000Res. 2017;6:760.View ArticlePubMedPubMed CentralGoogle Scholar

Copyright

© The Author(s) 2018

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. Please note that comments may be removed without notice if they are flagged by another user or do not comply with our community guidelines.

Advertisement