Open Access

Malaria hotspots defined by clinical malaria, asymptomatic carriage, PCR and vector numbers in a low transmission area on the Kenyan Coast

  • David Tiga Kangoye1Email author,
  • Abdisalan Noor1,
  • Janet Midega1,
  • Joyce Mwongeli1,
  • Dora Mkabili1,
  • Polycarp Mogeni1,
  • Christine Kerubo1,
  • Pauline Akoo1,
  • Joseph Mwangangi1,
  • Chris Drakeley2,
  • Kevin Marsh1, 3,
  • Philip Bejon1, 3 and
  • Patricia Njuguna1
Contributed equally
Malaria Journal201615:213

https://doi.org/10.1186/s12936-016-1260-3

Received: 18 December 2015

Accepted: 31 March 2016

Published: 14 April 2016

Abstract

Background

Targeted malaria control interventions are expected to be cost-effective. Clinical, parasitological and serological markers of malaria transmission have been used to detect malaria transmission hotspots, but few studies have examined the relationship between the different potential markers in low transmission areas. The present study reports on the relationships between clinical, parasitological, serological and entomological markers of malaria transmission in an area of low transmission intensity in Coastal Kenya.

Methods

Longitudinal data collected from 831 children aged 5–17 months, cross-sectional survey data from 800 older children and adults, and entomological survey data collected in Ganze on the Kenyan Coast were used in the present study. The spatial scan statistic test used to detect malaria transmission hotspots was based on incidence of clinical malaria episodes, prevalence of asymptomatic asexual parasites carriage detected by microscopy and polymerase chain reaction (PCR), seroprevalence of antibodies to two Plasmodium falciparum merozoite antigens (AMA1 and MSP1-19) and densities of Anopheles mosquitoes in CDC light-trap catches.

Results

There was considerable overlapping of hotspots by these different markers, but only weak to moderate correlation between parasitological and serological markers. PCR prevalence and seroprevalence of antibodies to AMA1 or MSP1-19 appeared to be more sensitive markers of hotspots at very low transmission intensity.

Conclusion

These findings may support the choice of either serology or PCR as markers in the detection of malaria transmission hotspots for targeted interventions.

Keywords

Malaria Hotspots Spatial scan statistic Antibodies Serology Asymptomatic parasitemia Transmission Targeted intervention

Background

“Malaria hotspots” are defined as geographical areas within a wider area of transmission in which the transmission intensity is significantly higher than the average level in the surrounding area of that setting and are widely observed in malaria endemic regions [1]. Stable and unstable hotspots have been reported in Kilifi [2] and they occur at various scales ranging from regional to homestead level [3].

Factors that are likely to determine the risk and spread of malaria include environmental factors such as temperature, altitude, distance to water bodies, wind direction, and urbanization [46]. They also include intrinsic human characteristics, such as red blood cell genetic polymorphisms, differential host attractiveness to Anopheles mosquitoes, fetal haemoglobin and dietary factors in early infancy, and extrinsic factors such as agricultural practices, socio-economic factors, housing, level of education and behaviour [715].

Hotspots represent an opportunity for targeted control interventions that are expected to be more efficient than untargeted interventions and ultimately benefit the whole community [16].

Challenges in the identification of hotspots of transmission include the choice of the transmission marker to measure, the choice of the geospatial method of detection, the choice of the scale of detection, when to detect them and how stable they are [16, 17]. Asymptomatic parasite carriage, clinical malaria episodes, vector biting intensities or antibody responses to selected malaria antigens have been proposed as potential markers of malaria transmission in detecting hotspots in areas of low to moderate transmission intensity [18]. The exploration of PCR and serology as transmission markers has been especially suggested in areas of unstable or very low transmission intensity [19, 20].

In the present study, simultaneous measurements of several malaria transmission indicators were carried out in an area of low transmission including clinical, parasitological, serological and entomological markers. These different markers were then used to detect malaria transmission hotspots, to examine the spatial overlapping of the specific hotspots and to analyse the correlations between the markers. Ultimately, this study aims at providing additional evidence that might guide the choice of markers to be used in the detection of malaria transmission hotspots.

Methods

Ethical approval

The Kenya Medical Research Institute (KEMRI) Ethical Review Committee approved the Mal055 study (SSC 1445) and the MTI study (SSC 2072). Study procedures were explained, and written informed consent was sought and obtained from each participant or his parents/guardians (for children) prior to any study procedure. The study was conducted according to the Declaration of Helsinki.

Study area, population and surveillance method

The data used in the present study were taken from studies in Kilifi county on the Kenyan Coast. There were two cohorts monitored, one for clinical episodes during 2 years of follow up and a second cohort monitored via cross-sectional surveys. The data were collected from January 2012 to December 2013 for the longitudinal monitoring and from July to September 2012 and May to July 2013 for the first and second cross-sectional surveys respectively.

831 children aged 5–17 months residing in 633 homesteads were recruited into a randomized, controlled malaria vaccine trial in which longitudinal monitoring of malaria episodes was done [21]. Febrile malaria episodes were detected by passive case detection as previously described [21]. Clinical malaria was defined as the presence of fever (axillary temperature ≥37.5 °C) or history of fever in the past 24 h and parasitaemia ≥2500/μL [22].

In the same study area, two cross-sectional surveys involving 800 individuals (children and adults) were conducted in 2012 and 2013. The distribution of this population by age group is shown in Additional file 1. The homesteads, in which these participants were residing (211 and 183 in 2012 and 2013 respectively), were selected among 2456 homesteads recorded in sub-locations of the study administrative area by simple random sampling. The households involved in the malaria vaccine study were excluded. The cross-sectional surveys were used to measure asymptomatic parasitaemia, by microscopy of thick and thin blood smears and by PCR as described elsewhere [23], and IgG specific antibody responses to Plasmodium falciparum merozoite antigens [the apical membrane antigen 1 (AMA1) and the 19 kDa C-terminal region of the merozoite surface protein 1 (MSP1-19)] as previously described [24]. Travel data were not recorded for any of these studies.

Data from an entomological study conducted in the same study area were also available for 2012 and 2013. Mosquito captures using CDC light traps were conducted in 150 sampled houses, chosen at random, at six rounds covering the dry season, the long and the short rains. Anopheles gambiae and Anopheles funestus were the major human malaria vectors captured in the study area. The homesteads involved in the entomological study were not the same as those sampled for the clinical surveillance of children, and this limited the possibility to examine the association between household level mosquito exposure and household level malaria incidence. Longitude and latitude data for each homestead involved in the clinical and entomological studies were recorded during the surveys using handheld Garmin eTrex Global Positioning System devices. The study area, along with the distribution of the different homesteads involved, is illustrated in Fig. 1.
Fig. 1

Study area. Panels a and b show respectively a map of Kenya with a focus on Kilifi County and a map of Kilifi County highlighting the study area. On panel c, each dot represents the location of a homestead. The colors uniquely identify the studies. The different sizes of the dots help distinguish very close homesteads

Detection of hotspots

Using the scan statistic method by Kulldorff [25], clusters of significantly higher risk of malaria than the remaining surrounding study area were detected using clinical, biological and entomological markers. The following markers were examined: clinical malaria, positive blood films, positive PCR tests, seropositivity to AMA1 and MSP1-19 and densities of Anopheles mosquitoes. The cut offs for seropositivity to AMA1 and MSP1-19 in normalized optical density were, respectively 0.132 and 0.108 in 2012, and 0.091 and 0.13 in 2013; they were determined using previously described methods [26]. The application of the scan statistic by SaTScan has been described previously [25]. Briefly, a scanning window (set to “circular” in the present analysis) is moved across the study area, and the maximum number of events that are captured by the window is recorded. The maximum window size was set to 30 % of the population at risk. Each of the different scanning windows was evaluated as a potential cluster by the calculation of a likelihood ratio test statistic based on the observed, expected and total number of cases. The corresponding p value is calculated using a Monte Carlo method.

To detect hotspots of clinical malaria cases, we used a discrete Poisson model where the cases were the clinical malaria cases detected in each homestead; population was defined as all monitored individuals residing in the corresponding homesteads. A Bernoulli probability model was used to detect hotspots of positive blood films, hotspots of positive PCR tests and hotspots of individuals seropositive for AMA1 and MSP1-19. Cases were defined as individuals with a positive test (blood film, PCR or ELISA) in each homestead; the controls were defined as the individuals with negative tests in the corresponding homesteads. A discrete Poisson model, in which the cases were the Anopheles mosquitoes captured in each house, was used to detect hotspots of Anopheles mosquitoes; the population was defined as one individual per house.

For each detected hotspot, a relative risk (RR) was computed. The RR is the magnitude of the risk of malaria for individuals residing within the hotspot compared with those residing outside the hotspot. It is calculated as the ratio of the estimated risk within the hotspot and the estimated risk in the surrounding area. The estimated risk is calculated as the number of observed cases divided by the number of expected cases if the null hypothesis was true i.e. if the distribution of cases was totally random. The threshold for statistical significance of the hotspots was set to 0.05.

Two hotspots overlap when the distance between their centres is smaller than the sum of their radii. The degree of overlapping of hotspots was estimated by calculating, for a given couple of hotspots, the ratio of the common surface area by the total surface area of the smallest hotspot. The common surface area (A) of the intersecting hotspots is given by the following formula [27]:
$$\begin{aligned} A =&\, r^{2 } \cos^{ - 1} \left(\frac{{d^{2} + r^{2} - R^{2} }}{2dr}\right) + R^{2} \cos^{ - 1} \left(\frac{{d^{2} - r^{2} + R^{2} }}{2dR}\right) \\ &\quad - \frac{1}{2}\sqrt {\left( { - d = r + R} \right)\left( {d + r - R} \right)\left( {d - r + R} \right)\left( {d + r + R} \right)} \end{aligned}$$
where R and r are the radii of the hotspots and d the distance between their centres. When the smallest hotspot is entirely covered by the bigger hotspot with no intersection or when two concentric hotspots exactly overlap, a ratio = 1 is assigned.

Observations with missing coordinates data were 4.5, 3 and <1 % for serological, entomological and clinical surveillance data respectively; they were dropped prior to any analysis. Missing data for Anopheles mosquito capture and AMA1/MSP1-19 serology were <1 % in the respective datasets.

Statistical analysis

To examine the distribution of the markers of malaria transmission, the data were summarized at homestead level by calculating sum of clinical malaria cases, sum of positive blood films, sum of positive PCR tests and geometric mean antibody titre.

The data were then aggregated using a raster map of the study area derived from a Kilifi county administrative map (see Additional file 2); the original shapefile was downloaded from [28]. The resolution of the raster surface was set to 0.9 km. At this resolution and for each marker, each homestead was assigned to a unique cell by computing the shortest distance between the index homestead and the surrounding grid points. The values of each of the markers at homestead level were then aggregated at grid cell level. The statistics used to aggregate the markers were the mean for counts of positive blood films and positive PCR tests, the weighted mean for count of clinical malaria cases and the weighted geometric mean for antibody titres. This aggregation was repeated for each year. The spatial correlations between these markers were examined using Spearman's rank correlation coefficient on the aggregated data. SaTScan™ v9.4.1 was used to detect the hotspots and Stata 13.1 for Windows, StataCorp LP was used to perform the data analysis and produce the maps.

Results

Malaria morbidity and transmission indicators in the study area

The clinical, parasitological, serological and entomological markers measured in these studies are summarized in Table 1. Malaria transmission intensity was low in 2012 with parasite rate by microscopy at 2 % in the general population, and declined further to 0.2 % in 2013. Similarly, there was a decline in densities of malaria vectors in the study area in 2013 with Anopheles mosquitoes captured in only 6 % of the surveyed houses compared with 24 % in 2012.
Table 1

Yearly summary of clinical, parasitological, serological and entomological markers in the study area

 

Year

2012

2013

Longitudinal study

Homesteads/population

633/831

633/831

Homesteads with malaria

65 (10.3 %)

22 (3.5 %)

Malaria cases

112 (13.5 %)

28 (3.4 %)

Cross-sectional studies

Homesteads/population

211/779

183/797

Homesteads with positive blood films

8 (3.8 %)

2 (1.1 %)

Homesteads with positive PCR tests

31 (14.7 %)

22 (12 %)

Prevalence asymptomatic infection (microscopy), (95 % CI)

2 % (1.2–3.2)

0.2 % (0.03–0.9)

Prevalence asymptomatic infection (PCR), (95 % CI)

6.2 % (4.6–8)

3.3 % (2.2–4.8)

Seroprevalence of antibodies to AMA1, (95 % CI)

36.1 % (32.7–39.5)

20.4 % (17.7–23.4)

Seroprevalence of antibodies to MSP1-19, (95 % CI)

19.9 % (17.1–22.9)

10.5 % (8.5–12.9)

Entomological surveys

Homesteads

145

142

Homesteads with Anopheles

35 (24 %)

8 (6 %)

Range of Anopheles captured/house

0–17

0–6

Total Anopheles captured

101

15

Total An. gambiae captured

85

5

Total An. funestus captured

16

10

Malaria hotspots in the study area

For clinical malaria, asymptomatic parasitaemia determined by microscopy and Anopheles mosquitoes captures, there were fewer positive cases in 2013 compared to 2012 (Table 1) and fewer hotspots were identified (Figs. 2, 3, 4). In 2013, the PCR and AMA1, but not MSP1-19, hotspots were reduced to 10 % and 21 % of their size in 2012 respectively (Figs. 5, 6, 7); the clinical malaria and mosquito vector hotspots were limited to single homesteads (Figs. 2, 4). There was one stable hotspot of clinical malaria (Fig. 2) in terms of position and size, limited to a single homestead, but the three other hotspots identified in 2012 were not identified in 2013. No hotspots of asymptomatic parasitaemia detected by microscopy was observed in 2013 (Fig. 3).
Fig. 2

Hotspots of clinical malaria cases. Each blue circle represents a statistically significant hotspot with its relative risk (RR) and p value displayed beside the circle

Fig. 3

Hotspots of asymptomatic malaria infections detected by light microscopy. Each blue circle represents a statistically significant hotspot with its relative risk (RR) and p value displayed beside the circle. No hotspot was identified in 2013

Fig. 4

Hotspots of Anopheles mosquitoes. Anopheles gambiae and Anopheles funestus were the only human malaria vector species captured during the survey. The orange and black circles represent the statistically significant hotspots of Anopheles mosquitoes in 2012 and 2013 respectively. Each hotspot is displayed with its malaria relative risk (RR) and p value

Fig. 5

Hotspots of asymptomatic malaria infections detected by polymerase chain reaction (PCR). Each blue circle represents a statistically significant hotspot with its relative risk (RR) and p value displayed beside the circle

Fig. 6

Hotspots of individuals seropositive to Plasmodium falciparum apical membrane antigen 1 (AMA1). Each blue circle represents a statistically significant hotspot with its relative risk (RR) and p value displayed beside the circle

Fig. 7

Hotspots of individuals seropositive to Plasmodium falciparum merozoite surface protein 1 (MSP1-19). Each blue circle represents a statistically significant hotspot with its relative risk (RR) and p value displayed beside the circle

The sampling of homesteads for the cross-sectional surveys differed between 2012 and 2013 (Fig. 1). However the hotspot of asymptomatic parasitaemia detected by PCR in 2012 overlapped 39 % of the one identified in 2013 (see Additional files 3 and 4). Moreover, globally, the hotspots of children seropositive to AMA1 overlapped 100 % and 38 % of the hotspots of children seropositive to MSP1-19 in 2012 and 2013 respectively. When the marker used was seropositivity to both AMA1 and MSP1-19, the hotspots detected in 2012 globally overlapped 100 % and 4.4 % of the hotspots of individuals seropositive to MSP1-19 and AMA1 respectively. In 2013, the pattern was reversed with the hotspot of children seropositive to both AMA1 and MSP1-19 overlapping 100 % and 57 % of hotspots of children seropositive to AMA1 and MSP1-19 respectively (see Additional file 5). There was one location in 2012 where the three types of serology hotspots (i.e. seropositive to AMA1, seropositive to MSP1-19 and seropositive to both AMA1 and MSP1-19) exactly overlapped each other (see Additional file 5).

Variable overlapping of hotspots of clinical and parasitological markers of transmission occurred in 2012 (see Additional files 6 and 7). Two hotspots of clinical malaria and two hotspots of Anopheles mosquitoes, limited to single-homesteads, did not overlap the hotspot determined by positive PCR tests. The hotspot of asymptomatic parasitaemia detected by microscopy was totally contained within the hotspot determined by positive PCR tests.

Although the data were collected from different samples of homesteads for the different markers, these homesteads were all contained within the same single study area. The different hotspots were visualized together to further investigate the extent of intersection and overlapping between them (see Additional file 8). Most hotspots concentrated in the southern part of the study area in 2012 and moved towards the northern part in 2013. Seventy-one and sixty-six percent of hotspots overlapped with each other in 2012 and 2013 respectively, irrespective of the markers. Considerable overlapping was observed between the different hotspots as detailed in Additional files 7 and 9. The substantial overlapping of the AMA1 hotspot with that of asymptomatic infections detected by PCR observed in 2012 was also observed in 2013 when the transmission declined further.

Spatial correlations between markers of malaria transmission

The distribution of the different markers is shown in Additional files 10 and 11. With the exception of Anopheles mosquito densities, weak to moderate statistically significant correlations were found between the other markers of transmission in 2012 when the markers were averaged at grid cell level (see Table 2 and Additional file 12). Clinical malaria was weakly correlated with positive blood films (r2 = 0.07) but not with any other marker. Serological markers were better correlated with asymptomatic parasitaemia detected by PCR (r2 > 0.29) than with asymptomatic parasitaemia detected by microscopy (r2 < 0.13). Asymptomatic parasitaemia detected by microscopy was correlated with asymptomatic parasitaemia detected by PCR (r2 = 0.26) and serological markers correlated with each other (r2 = 0.40). However, in 2013, when the transmission intensity declined further, the only statistically significant correlations observed were between asymptomatic parasitaemia detected by microscopy and positive PCR tests (r2 = 0.11), and between antibodies to MSP1-19 and Anopheles mosquitoes (r2 = 0.34) (Table 3).
Table 2

Correlations between malaria transmission markers in 2012 at 0.9 km resolution

 

Clinical malaria cases

Positive blood films

Positive PCR tests

Anti-AMA1 antibody titres

Anti-MSP1-19 antibody titres

Anopheles mosquitoes captured

Clinical malaria cases

1

     

266

     

Positive blood films

0.2672

1

    

266

292

    

<0.0001

     

Positive PCR tests

0.0328

0.5114

1

   

266

292

292

   

0.5944

<0.0001

    

Anti-AMA1 antibody titres

0.0215

0.2927

0.5413

1

  

41

42

42

43

  

0.8937

0.06

0.0002

   

Anti-MSP1-19 antibody titres

−0.0444

0.3509

0.5745

0.6338

1

 

41

42

42

43

43

 

0.7828

0.0227

0.0001

<0.0001

  

Anopheles mosquitoes captured

0.0929

 

0.0648

−0.2398

−0.0218

1

87

87

87

20

20

90

0.3923

 

0.5513

0.3086

0.9272

 

All markers are expressed as average per cell of a 0.9 km resolution grid superimposed on the study area. Positive blood films, positive PCR tests and Anopheles mosquitoes captured are expressed as mean/grid cell. Antibody titres are expressed as weighted geometric mean/grid cell. Clinical malaria cases are expressed as weighted mean/grid cell. For each pair of markers the table reports from top to bottom the correlation coefficient (rs), the number of grid cells (n) and the p value for rs

Table 3

Correlations between malaria transmission markers in 2013 at 0.9 km resolution

 

Clinical malaria cases

Positive blood films

Positive PCR tests

Anti-AMA1 antibody titres

Anti-MSP1-19 antibody titres

Anopheles mosquitoes captured

Clinical malaria cases

1

     

266

     

Positive blood films

−0.0165

1

    

266

292

    

0.7884

     

Positive PCR tests

0.057

0.3295

1

   

266

292

292

   

0.3544

<0.0001

    

Anti-AMA1 antibody titres

−0.0339

0.0516

0.002

1

  

22

22

22

22

  

0.8808

0.8196

0.9931

   

Anti-MSP1-19 antibody titres

−0.2376

0.0172

−0.0773

−0.0627

1

 

22

22

22

22

22

 

0.2869

0.9394

0.7323

0.7817

  

Anopheles mosquitoes captured

0.1693

−0.0343

0.116

0.1943

0.583

1

87

87

87

12

12

90

0.1169

0.7527

0.2846

0.5451

0.0467

 

All markers are expressed as average per cell of a 0.9 km resolution grid superimposed on the study area. Positive blood films, positive PCR tests and Anopheles mosquitoes captured are expressed as mean/grid cell. Antibody titres are expressed as weighted geometric mean/grid cell. Clinical malaria cases are expressed as weighted mean/grid cell. For each pair of markers the table reports from top to bottom the correlation coefficient (rs), the number of grid cells (n) and the p value for rs

Discussion

The present study describes the fine-scale spatial distribution of P. falciparum malaria, examining the relationships between different markers of malaria transmission in an area on the coast of Kenya. The levels of malaria transmission markers seen in this study were lower in 2013 compared with 2012. The low number of asymptomatic infections detected by microscopy prevented us having enough power to detect hotspots in 2013, but we could still detect hotspots with the larger number of positives seen by PCR. Most of the hotspots were unstable (i.e. inconsistent in location between 2012 and 2013), but one hotspot of clinical malaria was maintained in its position and size over the 2 years. When the transmission intensity declined, the spatial correlations observed between the markers were reduced to correlations between parasitological markers on the one hand, and serological and entomological markers on the other hand.

The decline of malaria transmission observed in the present study seems opposite to the observed trends of P. falciparum parasite rates along the coast [29]. However, this study was conducted in a restricted area and previous studies have reported high rates of heterogeneity in malaria transmission in the region, and that differing trends can be observed in sub-locations within the same area [3].

From 2012 to 2013, 57 % of hotspots disappeared and among the remaining ones, only PCR and serology hotspots maintained a size above the homestead level; the other hotspots shrank to single homesteads. Hotspots of asymptomatic parasite carriers detected by microscopy were not seen in 2013 despite ongoing transmission evidenced by clinical malaria cases. This suggests that cross-sectional surveys using microscopy may not be ideal when transmission intensity declines to very low levels [30]. The hotspots that persisted were asymptomatic parasite carriers detected by PCR and serological methods, suggesting these markers as good candidates for sensitive hotspot detection in settings with declining malaria transmission.

In 2012, there was a total overlap of hotspots of asymptomatic parasite carriers detected by microscopy with hotspots of asymptomatic parasite carriers detected by PCR as expected, especially given that the sensitivity of PCR is higher than that of light microscopy [31]. This is consistent with the statistically significant spatial correlation observed between these markers when the data were analysed at grid cell level. On the other hand, epidemiological studies have shown that parasite density can be inversely proportional to the intensity of transmission at a micro-epidemiological scale [32], and this might have led microscopy-defined hotspots to be differently located from PCR-defined hotspots. In the present study the transmission intensity was much lower and this phenomenon was not observed. The hotspots of asymptomatic parasite carriers detected by PCR overlapped the hotspots detected by serological markers in 2012 and 2013, supporting the idea of using serological markers as an alternative to PCR in the detection of hotspots. It has been shown previously that children living in hotspots of asymptomatic parasitaemia have higher antibody titres compared with those living in clinical malaria hotspots [2], and antibody titres have been described as a marker of exposure [33].

One clinical malaria hotspot was found to be stable across the 2 years, which is not consistent with previous reports in which hotspots of clinical malaria were found to be unstable compared with hotspots of asymptomatic parasitaemia [2]. However, the short period of observation in the present study and the low age of children assessed (i.e. 5–17 months olds) in a low transmission setting are the likely explanation of this observation since immunity to clinical malaria builds up over a much longer period at lower transmission intensities [34, 35].

The relative simplicity and lower cost of serology compared with PCR may make the use of serological markers more attractive for large-scale surveillance. However the fact that serological surveys may not distinguish recent from medium-term exposure may be a disadvantage, since the location of hotspots may vary from year to year. This could be overcome by including only young children in the surveys [36] whose antibody responses have been attributed to short-lived plasma cells [37, 38] or by measuring responses to antigens for which evidence suggest that they have limited capacity to induce long-lived plasma cells [39]. Helb et al. have recently reported that antibody responses to some novel malaria antigens can limit detection to infections occurring within the last 30 days [40].

The present study was opportunistic based on the availability of datasets and thus presents with some limitations. The sampled homesteads were not the same for the entomological, serological and clinical surveillance studies and this prevents us from examining homestead-level correlations in more detail. The sample size was not large and the limited period of observation does not allow a definitive assessment of temporal stability.

Conclusions

The global decline of malaria transmission and plans for elimination have led to increased interest in the fine-scale epidemiology of malaria. One of the challenges in targeted interventions is the appropriate detection of residual transmission foci at the pre-elimination stage. The choice of a cost-effective marker that can be logistically feasible and readily implemented across sites by malaria control programmes would be important in the elimination efforts as well as the post-elimination surveillance. These findings may support the choice of either serology or PCR as markers in the detection of transmission hotspots for targeted interventions.

Availability of supporting data

The supporting data are under the custodianship of the KEMRI-Wellcome Trust Data Governance Committee and is accessible upon request addressed to that committee.

Notes

Abbreviations

AMA1: 

apical membrane antigen 1

CDC: 

Centers for Disease Control and Prevention

ELISA: 

enzyme-linked immunosorbent assay

KEMRI: 

Kenya Medical Research Institute

MSP1-19: 

merozoite surface protein 1

PCR: 

polymerase chain reaction

RR: 

relative risk

Declarations

Authors’ contributions

Conceived and designed the experiments: JMi, JMwa, CD, KM, PB. Obtained ethical approval for completion of study: PN. Recruited volunteers for study: CK, PA, PN. Performed the experiments: JMwo, DM. Analysed the data: DK, AN, PB, PM. Drafted or revised the article: DK, AN, JMi, JMwo, DM, PM, CK, PA, CD, JMwa, KM, PB, PN. All authors read and approved the final manuscript.

Acknowledgements

Work was funded by PATH-Malaria Vaccine Initiative. PB was jointly funded by the UK Medical Research Council (MRC) and the UK Department for International Development (DFID) under the MRC/DFID Concordat agreement. The Wellcome Trust supports infrastructure in Kilifi (Grant number B9RTIR0). The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript. Permission to submit the manuscript for publication was given by the Director of the Kenya Medical Research Institute.

Competing interests

Prof. Chris Drakeley is an Associate Editor of Malaria Journal.

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)
Kenya Medical Research Institute-Wellcome Trust Research Programme, Centre for Geographic Medicine Research
(2)
Department of Infectious and Tropical Diseases, London School of Hygiene and Tropical Medicine
(3)
Nuffield Department of Medicine, Centre for Clinical Vaccinology and Tropical Medicine, Churchill Hospital, University of Oxford

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© Kangoye et al. 2016

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