Plasmodium vivax has been proposed to infect and replicate in the human spleen and bone marrow. Compared to Plasmodium falciparum, which is known to undergo microvascular tissue sequestration, little is known about the behavior of P. vivax outside of the circulating compartment. This may be due in part to difficulties in studying parasite location and activity in life.
Methods and findings
To identify organ-specific changes during the early stages of P. vivax infection, we performed 18-F fluorodeoxyglucose (FDG) positron emission tomography/magnetic resonance imaging (PET/MRI) at baseline and just prior to onset of clinical illness in P. vivax experimentally induced blood-stage malaria (IBSM) and compared findings to P. falciparum IBSM. Seven healthy, malaria-naive participants were enrolled from 3 IBSM trials: NCT02867059, ACTRN12616000174482, and ACTRN12619001085167. Imaging took place between 2016 and 2019 at the Herston Imaging Research Facility, Australia. Postinoculation imaging was performed after a median of 9 days in both species (n = 3 P. vivax; n = 4 P. falciparum). All participants were aged between 19 and 23 years, and 6/7 were male. Splenic volume (P. vivax: +28.8% [confidence interval (CI) +10.3% to +57.3%], P. falciparum: +22.9 [CI −15.3% to +61.1%]) and radiotracer uptake (P. vivax: +15.5% [CI −0.7% to +31.7%], P. falciparum: +5.5% [CI +1.4% to +9.6%]) increased following infection with each species, but more so in P. vivax infection (volume: p = 0.72, radiotracer uptake: p = 0.036). There was no change in FDG uptake in the bone marrow (P. vivax: +4.6% [CI −15.9% to +25.0%], P. falciparum: +3.2% [CI −3.2% to +9.6%]) or liver (P. vivax: +6.2% [CI −8.7% to +21.1%], P. falciparum: −1.4% [CI −4.6% to +1.8%]) following infection with either species. In participants with P. vivax, hemoglobin, hematocrit, and platelet count decreased from baseline at the time of postinoculation imaging. Decrements in hemoglobin and hematocrit were significantly greater in participants with P. vivax infection compared to P. falciparum. The main limitations of this study are the small sample size and the inability of this tracer to differentiate between host and parasite metabolic activity.
PET/MRI indicated greater splenic tropism and metabolic activity in early P. vivax infection compared to P. falciparum, supporting the hypothesis of splenic accumulation of P. vivax very early in infection. The absence of uptake in the bone marrow and liver suggests that, at least in early infection, these tissues do not harbor a large parasite biomass or do not provoke a prominent metabolic response. PET/MRI is a safe and noninvasive method to evaluate infection-associated organ changes in morphology and glucose metabolism.
Why was this study done?
- In contrast to Plasmodium falciparum, blood-stage Plasmodium vivax is not traditionally thought to accumulate outside of the circulating blood compartment.
- Emerging data suggest that a hidden compartment of P. vivax may exist outside of circulation, in reticulocyte (very young red blood cells)-containing organs.
- The presence of a hidden compartment affects our understanding of the basic biology and pathology of this common parasite and may have implications when developing antimalarial treatments.
- Studying the accumulation of malaria parasites is extremely challenging in vivo and has historically been limited to late stage disease and postmortem studies.
What did the researchers do and find?
- We performed whole body magnetic resonance imaging (MRI) and positron emission tomography (PET) in individuals undergoing experimental malaria infection to identify changes in organ morphology and glucose metabolism following infection.
- Splenic uptake of radiolabeled glucose increased following P. vivax and P. falciparum infection and was more pronounced in the P. vivax group.
- Glucose uptake in the liver and bone marrow was not increased following infection with either P. vivax or P. falciparum.
What do these findings mean?
- Increased splenic glucose metabolism is present in the early stages of infection with both P. vivax and P. falciparum and is more pronounced in P. vivax, consistent with other emerging evidence of a greater predilection for the spleen in P. vivax than P. falciparum.
- Functional medical imaging may be a useful tool to study biological processes in experimental malaria infection.
Citation: Woodford J, Gillman A, Jenvey P, Roberts J, Woolley S, Barber BE, et al. (2021) Positron emission tomography and magnetic resonance imaging in experimental human malaria to identify organ-specific changes in morphology and glucose metabolism: A prospective cohort study. PLoS Med 18(5):
Academic Editor: Lorenz von Seidlein, Mahidol-Oxford Tropical Medicine Research Unit, THAILAND
Received: September 19, 2020; Accepted: February 17, 2021; Published: May 26, 2021
Copyright: © 2021 Woodford et al. This is an open access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Data Availability: Raw imaging files are electronically tagged with personally identifiable information and cannot be shared publicly to protect the confidentiality of participants. All other data are within the manuscript and its Supporting Information files.
Funding: This project was supported by a HIRF Seed Funding Grant, Metro North Hospital and Health Service (J.W) and by the Australian National Health and Medical Research Council (J.S.M #1135955, #1037304, #1132975, and N.M.A #1135820, 1098334). The clinical trials contributing participants were funded by the Australian National Health and Medical Research Council (J.S.M #1132975), the Bill and Melinda Gates Foundation (J.S.M OPP1111147) and the Global Health Innovative Technology Fund. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
confidence interval; FDG,
18-F fluorodeoxyglucose; IBSM,
induced blood-stage malaria; iRBC,
infected red blood cell; MRI,
magnetic resonance imaging; PET,
positron emission tomography; qPCR,
quantitative polymerase chain reaction; ROI,
region of interest; STROBE,
Strengthening The Reporting of OBservational Studies in Epidemiology; SUV,
standardized uptake value; ULN,
upper limit of normal
Plasmodium vivax and Plasmodium falciparum have key differences in their biology, pathophysiology, and disease manifestations. These are thought to largely arise from differences in microvascular parasite sequestration [1–3] and host red blood cell tropism, with P. vivax having a strict tropism for immature reticulocytes [4,5]. Differences in organ-specific parasite tropism have also been proposed . Although P. vivax is not thought to undergo significant microvascular tissue sequestration, there is emerging evidence that the spleen may harbor a large hidden reservoir of replicating parasites [6,7]. The evaluation of sequestration and organ-specific parasite tropism has largely relied on biochemical markers, nonhuman primate models, and postmortem studies, which have been critical to progress our understanding of disease pathophysiology but are imperfect tools to study the dynamics of infection in humans.
The tissue distribution of P. falciparum on autopsy has been well described. In a seminal publication by Marchiafava and Bignami, the greatest concentration of schizonts was found in the brain, followed by the lungs, spleen, bone marrow, liver, and intestines . Although human autopsy studies of P. vivax are comparatively rare, parasite material has been identified in the spleen, liver, and lungs, but not the brain . Studies of P. vivax tropism in nonhuman primates have been limited by the need for prior splenectomy . In these studies, few or no parasites were identified in the brain or intestines, whereas the bone marrow and liver sinusoids were major tissue reservoirs for P. vivax schizonts and gametocytes . An apparent predilection for the spleen, bone marrow, and liver is consistent with biomarker evidence of a hidden biomass of parasite accumulating in non-endothelial lined spaces  and the strict reticulocyte tropism of this species, which may promote concentration in organs in which immature reticulocytes accumulate [4,11]. Nonetheless, this hypothesis is challenging to confirm in life, where these processes are largely inaccessible to evaluation. In this context, magnetic resonance imaging (MRI) and functional imaging using nuclear medicine such as positron emission tomography (PET) may be useful noninvasive methods to study deep tissue processes and organ-specific tropism, particularly in early and non-severe infection.
As access to clinical imaging infrastructure in malaria endemic areas continues to improve, an increasing number of studies have demonstrated the utility of MRI to evaluate the brain in cerebral  and uncomplicated falciparum malaria [13,14]. In contrast, PET imaging in malaria is limited to a small number of nonhuman primate studies [15,16] and a single case report of serendipitous imaging in suspected lymphoma . In the nonhuman primate studies, uptake of the glucose biomimetic 18-F fluorodeoxyglucose (FDG) was colocated with sequestered infected red blood cells (iRBCs) as ascertained on subsequent autopsy , suggesting that PET imaging using this widely available radiotracer that targets glucose utilization may be a useful modality to localize organ-specific parasite accumulation and host response in life.
We sought to investigate organ-specific changes in morphology and glucose metabolism in the spleen, vertebral bone marrow, and liver in early P. vivax and P. falciparum infection using FDG PET/MRI imaging of participants with experimentally induced blood-stage malaria (IBSM). We hypothesized that alterations in glucose metabolism would be present in the regions of interest (ROIs). Secondly, we hypothesized that the patterns of PET/MRI would differ between participants with P. vivax and P. falciparum infection.
This was a prospective, single-center exploratory study performed between 2016 and 2019 at the Herston Imaging Research Facility, Brisbane, Australia. Participants were recruited to the imaging study after enrolling in IBSM studies. In brief, baseline FDG PET/MRI was performed prior to malaria inoculation. Healthy, malaria-naive participants were then inoculated with approximately 564 viable P. vivax or approximately 2,800 P. falciparum (3D7) infected erythrocytes. Peripheral blood parasitemia was monitored at least daily by quantitative polymerase chain reaction (qPCR) from day 4 after inoculation as described previously . A postinoculation FDG PET/MRI was performed near to the peak of parasitemia, in the 24 hours prior to administration of antimalarial treatment. Standard safety assessments including clinical review, hematology, and biochemistry parameters were performed at specified times during the IBSM studies including baseline, 1 day following postinoculation imaging (at time of treatment), and in convalescence, 1 to 2 weeks after postinoculation imaging [19,20]. A total of 8 participants were planned for enrollment, based on the availability of funding, IBSM study cohorts, and imaging facilities.
Baseline and postinoculation FDG PET/MRI were performed on all participants using the 3 Tesla Magnetom Biograph mMR (Siemens, Erlangen, Germany). All participants completed an institutional MRI safety checklist prior to imaging. The female participants underwent qualitative human chorionic gonadotropin testing prior to imaging to exclude pregnancy. Participants were required have a normal fasting glucose at enrolment and to abstain from strenuous exercise and follow a low-carbohydrate diet in the 24 hours prior to imaging with a 6-hour fasting period immediately prior to help standardize FDG uptake [21,22]. Diet and activity information sheets were provided to assist participant adherence. Due to the different growth rate of parasites in IBSM, the interval between baseline and postinoculation imaging differed in the P. vivax and P. falciparum studies.
Nuclear medicine and radiology specialists reporting all imaging were not aware of the inoculum species. Mean standardized uptake values (SUVs) were estimated for the prespecified ROIs including the spleen, vertebral bone marrow, and liver. SUV is the most commonly used measurement of radiotracer activity and represents the ratio of tissue radioactivity related to FDG at a given time and the injected dose of radioactivity per kilogram of participant weight. Organ volumes were calculated for the spleen and liver. As an exploratory analysis, the quantitative rate of irreversible radiotracer uptake was modeled for the ROIs. Detailed methods and imaging protocols are outlined in the S1 Text.
All imaging results are presented descriptively for the P. vivax and P. falciparum groups. Where relevant, results for each inoculum group are presented as mean (95% confidence interval (CI)) percentage change from baseline for quantitative imaging metrics. A >10% percentage difference in SUV from baseline to postinoculation imaging was considered meaningful based on intraindividual, inter-scan variability reported in stringent FDG PET imaging trials in malignancy and non-malignancy settings [23–25]. Parasitemia at the time of postinoculation imaging was estimated by interpolating the linear rate of change between the nearest log-transformed study parasitemia measurements.
Statistical analysis was performed using Prism 8.4.2 (GraphPad, San Diego, United States of America). In an exploratory analysis, baseline and postinoculation imaging metrics and selected hematology and biochemistry parameters were compared using paired, 2-tailed t tests. Differences between the mean percentage change from baseline for quantitative imaging metrics for P. vivax and P. falciparum groups were compared using unpaired t tests. Differences between selected hematology and biochemistry parameters and parasitemia measurements for P. vivax and P. falciparum groups were compared using unpaired t tests of Mann–Whitney U tests. A p-value <0.05 was considered significant. No adjustments have been made for multiple comparisons.
Participants were recruited from 3 IBSM studies: 2 published (P. falciparum: NCT02867059  and P. vivax: ACTRN12616000174482 ) and 1 unpublished (P. falciparum: ACTRN12619001085167). These studies were approved by the QIMR-Berghofer Medical Research Institute Ethics Committee. The exploratory imaging study was approved by the QIMR-Berghofer Medical Research Institute and Queensland Health Metro North Ethics committees. The exploratory imaging study was prospectively linked to 2 of the IBSM studies (ACTRN12616001458426 linked to IBSM study NCT02867059 and ACTRN12616001238460 linked to IBSM study ACTRN12616000174482 (see S1 Protocol)). The third IBSM study incorporated the exploratory imaging study into the main protocol (ACTRN12619001085167). All participants provided written informed consent for the IBSM studies and the exploratory imaging study. This study has been reported as per the Strengthening The Reporting of OBservational Studies in Epidemiology (STROBE) guidelines (S1 Checklist).
A total of 8 healthy, malaria-naive participants were recruited. All participants underwent baseline imaging within 7 days before inoculation. One participant was enrolled and underwent baseline imaging, but was excluded from the IBSM study before inoculation due to incidental hypokalemia on baseline biochemistry. This participant did not undergo postinoculation imaging and was excluded from the analysis. Seven participants underwent postinoculation imaging. The study population is described in Table 1. Included participants had a median age of 20 years (range 19 to 23), and 6/7 were male. Three were inoculated with P. vivax and 4 with P. falciparum. All participants developed a measurable parasitemia (Fig 1) and reported symptoms of early malaria infection prior to treatment. Parasitemia at postinoculation imaging was at least as high in the P. falciparum group (median 22,326 [range 998 to 99,134 parasites/mL]) as the P. vivax group (median 6,042 [range 5,818 to 29,097 parasites/mL, Mann–Whitney U test p > 0.99]). Although the day of treatment varied between studies, both groups underwent imaging a median 9 days following inoculation. Imaging results for the ROIs including organ volumes and SUVs are presented in Fig 2 and S1 Table. Exploratory calculation of the quantitative rate of radiotracer uptake for the ROIs is presented in the S1 Table and S2 Text.
Fig 2. Imaging indices at baseline and postinoculation.
(A) Spleen (volume), (B) Liver (volume), (C) Spleen (SUV), (D) Liver (SUV), and (E) Vertebral Bone Marrow (SUV). P. vivax group represented by black lines with unfilled markers. P. falciparum group represented by gray lines with filled markers. Asterisk represents p < 0.05 in paired t test comparison with baseline measurements (black for P. vivax, gray for P. falciparum). SUV, standardized uptake value.
In the P. vivax group, splenic SUVs increased +15.5% from baseline (CI −0.7% to +31.7%). SUVs on postinoculation imaging were significantly higher on postinoculation imaging compared to baseline imaging (paired t test p = 0.044). This was visible on qualitative review in some participants (Fig 3). Splenic volume increased a mean +28.8% from baseline imaging but did not reach statistical significance (CI +0.3% to +57.3%, paired t test p = 0.053).
Fig 3. Baseline and postinoculation PET imaging in Participant 1 (P. vivax group).
Increased radiotracer uptake is evident in the spleen on postinoculation imaging (arrowhead). PET, positron emission tomography.
In the P. falciparum group, splenic SUVs increased +5.5% from baseline (CI +1.4% to +9.6%, paired t test p = 0.019), less than the prespecified 10% threshold. Splenic volume increased +22.9% from baseline but did not reach statistical significance (CI −15.3% to +61.1%, paired t test p = 0.20.) Participant 4 demonstrated a slight reduction in splenic volume, contrary to all other participants.
Compared to the P. falciparum group, the P. vivax group demonstrated a greater increase in splenic SUV from baseline to postinoculation imaging (+15.5% [CI −0.7% to +31.7%] versus +5.5% [CI +1.4% to +9.6%], unpaired t test p = 0.036). The change in splenic volume was larger in the P. vivax group compared to the P. falciparum group but did not reach statistical significance (+28.8% [CI +0.3% to +57.3%] versus +22.9% [CI −15.3% to +61.1%], unpaired t test p = 0.72).
Vertebral bone marrow imaging
Vertebral bone marrow SUVs were stable on postinoculation imaging in both the P. vivax group (+4.6% [CI −15.9% to +25.0%], paired t test p = 0.44) and the P. falciparum group (+3.2% [CI −3.2% to +9.6%], paired t test p = 0.17). Participant 2 (P. vivax group) was the only individual demonstrating a change in SUV above the prespecified 10% threshold. There was no significant difference in change in percentage change in SUV between the groups (unpaired t test p = 0.77).
In both the P. vivax and P. falciparum groups, hepatic volume and SUVs remained stable on postinoculation imaging (P. vivax: hepatic volume: +0.2% [CI −23.6% to +24.0%], paired t test p = 0.84; SUV: +6.2% [CI −8.7% to +21.1%], paired t test p = 0.18; P. falciparum: hepatic volume: +3.9% [CI −6.2% to 14.0%], paired t test p = 0.32; SUV: −1.4% [CI −4.6% to +1.8%], paired t test p = 0.25). Participant 2 (P. vivax group) was the only individual demonstrating a change in SUV above the prespecified 10% threshold.
There was no significant difference in hepatic volume change or SUV change between the groups (percentage change in volume unpaired t test p = 0.56 and SUV unpaired t test p = 0.06).
Safety, clinical review, and laboratory parameters
No imaging-related adverse events or incidental radiological findings requiring clinical follow-up were recorded. All participants experienced symptoms of early malaria infection. Non-tender palpable splenomegaly was reported in Participant 3 following P. vivax inoculation on routine examination performed on the day of postinoculation imaging. This was present on inspiration, extended 1 cm below the costal margin, and resolved on follow-up examination 3 days following postinoculation imaging. Clinical hepatomegaly or splenomegaly was not reported for the remaining participants in either group.
Routine hematology (hemoglobin, hematocrit, and platelet count) and biochemistry (total bilirubin and alanine transaminase) measurements were collected at baseline, postinoculation (at time of treatment), and in convalescence for all participants. The majority of hematology and biochemistry measurements were within the laboratory reference range (S1 Fig, S2 Table). Changes in laboratory parameters in our study population were similar to those observed in the overall contributing IBSM study populations [26,27].
In the P. vivax group, hemoglobin and hematocrit decreased significantly between baseline and postinoculation (mean 148 g/L [CI 103 to 193] versus 137 g/L [CI 94 to 180], paired t test p = 0.045 and 0.43 L/L [CI 0.33 to 0.53] versus 0.39 L/L [CI 0.28 to 0.50], paired t test p = 0.008, respectively) and further at convalescence (148 g/L [CI 103 to 193] versus 133 g/L [CI 85 to 182], paired t test p = 0.004 and 0.43 L/L [CI 0.33 to 0.53] versus 0.38 L/L [CI 0.25 to 0.51], paired t test p = 0.020). Platelets decreased at postinoculation (206 × 109/L [CI 172 to 241] versus 134 × 109/L [CI 109 to 159], paired t test p = 0.034) and increased slightly compared to baseline at convalescence, but did not reach statistical significance (206 × 109/L [CI 172 to 241] versus 218 × 109/L [range 211 to 226], paired t test p = 0.28). There were no statistically significant changes in biochemistry measurements between baseline and postinoculation or between baseline and convalescence (S2 Table), although Participant 1 experienced a clinically relevant elevation in alanine transaminase in convalescence (Day 17, 86 IU/L, 2.2 ×upper limit of normal (ULN)). In the P. falciparum group, there were no statistically significant changes in hematology or biochemistry measurements between baseline and postinoculation or between baseline and convalescence (S2 Table). Participants 5, 6, and 7 each experienced elevated alanine transaminase measurements in convalescence (85 IU/L, 2.1 ×ULN; 73 IU/L, 1.8 ×ULN; 128 IU/L, 3.2 ×ULN, respectively).
Compared to the P. falciparum group, the hemoglobin decrease was greater from baseline to postinoculation in the P. vivax group (mean −7.2% [CI −13.4% to −1.1%] versus +1.2% [CI −1.3% to +3.8%], unpaired t test p = 0.003). This was similar for hematocrit (−8.7% [CI −13.5% to −3.9%] versus −2.3% [CI −6.4% to +1.9%], unpaired t test p = 0.017). Conversely, decrease in platelet count was greater from baseline to convalescence in the P. falciparum group compared to the P. vivax group (−33.5% [CI −69.5% to +2.5%] versus +5.9% [CI −10.7% to +22.6%], unpaired t test p = 0.035). There were no other differences between the groups in any other changes in hematology or biochemistry measurements.
We demonstrate that medical imaging using PET and MRI are technically feasible and safe in experimental human P. vivax and P. falciparum infection and can define organ-specific physiological changes very early in disease. The increase in splenic volume and utilization of glucose on postinoculation imaging was most pronounced in the P. vivax group. Although the sample size is small, in the exploratory statistical comparisons, increase in splenic SUV was significantly greater in participants with P. vivax compared to those with P. falciparum. These findings suggest splenic tropism with both species early in the course of disease, but that it is significantly greater for P. vivax compared to P. falciparum.
Changes in splenic imaging metrics may be associated with either increased parasite or host activity, or a combination of both. This is consistent with nonhuman primate Plasmodium coatneyi infection studies, where increased splenic FDG uptake associated with accumulation of iRBCs in the red pulp and lymphoid hyperplasia have been reported . In vitro studies have shown that iRBCs consume up to 100 times the amount of glucose than that consumed by uninfected erythrocytes  and that trophozoite uptake is up to 6-fold greater than that of ring stages . While no Plasmodium studies have been performed to identify if this in vitro glucose consumption is sufficient to be detected by FDG PET, the principle of clinically detectable tracer uptake by pathogens has been demonstrated in bacteria . Taken together, these findings may suggest that splenic FDG signal reflects iRBC accumulation within the spleen.
The spleen has been proposed as a site for accumulation of P. vivax infection [3,6,10,31]. The extent to which this occurs in early infection and in clinical disease is not clear. Indirect evidence points to accumulation of non-phagocytosed P. vivax iRBCs in the spleen in acute malaria [4,10], with supporting direct evidence from case reports [6,32]. Furthermore, early splenic rupture may occur more frequently in P. vivax compared to P. falciparum infection , which may suggest a greater tropism of this species for the spleen. In an ex vivo perfused spleen model, a subpopulation of P. falciparum ring stage parasites are retained in the red pulp of the spleen , hypothesized as mechanism to reduce acute host morbidity and prolong the duration of transmissible infection . In a nonhuman primate P. vivax model, spleen-dependent expression of molecules mediating adhesion to human splenic fibroblasts has been described , suggesting the presence of a parasite phenotype that may favor splenic accumulation. Finally, very recent data suggest that immature reticulocytes accumulate in the human spleen providing a favorable niche for P. vivax accumulation . We now show evidence supporting splenic tropism and splenic accumulation of P. vivax very early in infection.
Both P. falciparum [1,37] and P. vivax [9,38] have also been shown to infect the bone marrow. The lack of signal change in the vertebral bone marrow suggest that this tissue may have a lower parasite biomass in early infection, or alternatively, that parasites located in the bone marrow do not provoke as prominent host metabolic response. This is in keeping with a recent study suggesting that in acute vivax malaria, the parasite concentration in the bone marrow is, on average, no higher than that circulating in peripheral blood .
Similarly, while P. falciparum  and P. vivax  have been found in liver at autopsy, the absence of volume or tracer signal change in our study suggests that this may not be a site of accumulation early in infection. In our cohort, participants from both the P. vivax and P. falciparum groups experienced elevated transaminases in convalescence. Elevated transaminases following treatment have been previously described in experimental P. vivax , P. falciparum  infections, and in naturally acquired infection in non- or pauci-immune patients [39,41] and are unlikely to be related to imaging, but rather may be related to inflammation and hemolysis .
The P. vivax group experienced a greater decrease in hematology indices from baseline to postinoculation compared to the P. falciparum group. The greater removal of RBCs from circulation previously described in P. vivax infection compared to P. falciparum infection is thought to occur in the spleen , which may also contribute to the imaging findings. Reduction in platelets in experimental malaria has been previously described and may relate to splenic pooling or more generalized platelet removal from circulation due to endothelial activation or parasite killing . We and others have previously described the association between endothelial activation and thrombocytopenia in experimental malaria [44,45], and labeled, auto-transfused platelets have been observed to undergo disseminated extra-splenic consumption in uncomplicated P. falciparum infection .
There were several limitations to this study. The population of the study was small, and statistical comparisons of baseline imaging to postinoculation imaging are necessarily of an exploratory nature, as there is limited power to discriminate between groups. Secondly, while FDG is a readily available radiotracer, it is relatively nonspecific and is unable to differentiate between host and parasite activity. Advances in radiochemistry may permit the development of a radiotracer with sufficient specificity to selectively image iRBCs. Finally, we were unable to control for other variables that may have influenced the differences observed between the groups such as parasitemia at the time of imaging.
To date, the ability to localize the pathology of malaria in life has been limited, and direct evaluation of sequestration and organ-specific parasite tropism has relied upon animal models and postmortem studies. Using the IBSM model, we have demonstrated that the medical imaging techniques MRI and PET may be used to study human P. vivax and P. falciparum infection in life and observe early infection in a way not previously possible. The presence of alterations in splenic glucose uptake and volume soon after blood-stage infection compared to baseline suggests that these imaging techniques may be useful to localize disease. The differences observed between species consolidates the concept of species-specific tissue tropism, where P. vivax has a greater predilection for the spleen. Our findings suggest that the hypothesized endosplenic life cycle of P. vivax may be established soon after blood-stage infection.
We would like to thank Louise Campbell and Peta Gray from HIRF for their help in coordinating the imaging of participants and Dr. Manoj Bhatt at the Department of Nuclear Medicine, RBWH for serving as the imaging medical monitor; Marita Prior at the Department of Radiology, RBWH for her help in coordinating the reporting of imaging; study staff at Q-Pharm Pty Ltd for their help in coordinating the IBSM participant exploratory study involvement; Medicines for Malaria Venture for encouraging investigator-initiated studies; and all participants for volunteering their time.
Marchiafava E, Bignami A. On summer-autumnal fever. London: New Sydenham. Society. 1894.
Bass CC. An Attempt to Explain the Greater Pathogenicity of Plasmodium Falciparum as Compared with Other Species. Am J Trop Med Hyg. 1921;s1-1(1):29–33. https://doi.org/10.4269/ajtmh.1921.s1-1.29
Baird JK. Evidence and Implications of Mortality Associated with Acute Plasmodium vivax Malaria. Clin Microbiol Rev. 2013;26(1):36–57. PubMed Central PMCID: PMC23297258. pmid:23297258
Malleret B, Li A, Zhang R, Tan KSW, Suwanarusk R, Claser C, et al. Plasmodium vivax: restricted tropism and rapid remodeling of CD71-positive reticulocytes. Blood. 2015;125(8):1314–24. pmid:25414440
Gruszczyk J, Kanjee U, Chan L-J, Menant S, Malleret B, Lim NTY, et al. Transferrin receptor 1 is a reticulocyte-specific receptor for Plasmodium vivax. Science. 2018;359(6371):48–55. pmid:29302006
Machado Siqueira A, Lopes Magalhaes BM, Cardoso Melo G, Ferrer M, Castillo P, Martin-Jaular L, et al. Spleen rupture in a case of untreated Plasmodium vivax infection. PLoS Negl Trop Dis. 2012;6(12):e1934. pmid:23272256; PubMed Central PMCID: PMC3521714.
Kho S, Qotrunnada L, Leonardo L, Andries B, Wardani P, Fricot A, et al. Hidden biomass of intact malaria parasites in the human spleen. N Engl J Med. Forthcoming 2021.
Lacerda MV, Fragoso SC, Alecrim MG, Alexandre MA, Magalhaes BM, Siqueira AM, et al. Postmortem characterization of patients with clinical diagnosis of Plasmodium vivax malaria: to what extent does this parasite kill? Clin Infect Dis. 2012;55(8):e67–74. pmid:22772803.
Obaldia N 3rd, Meibalan E, Sa JM, Ma S, Clark MA, Mejia P, et al. Bone Marrow Is a Major Parasite Reservoir in Plasmodium vivax Infection. MBio. 2018;9(3). pmid:29739900; PubMed Central PMCID: PMC5941073.
Barber BE, William T, Grigg MJ, Parameswaran U, Piera KA, Price RN, et al. Parasite biomass-related inflammation, endothelial activation, microvascular dysfunction and disease severity in vivax malaria. PLoS Pathog. 2015;11(1):e1004558. pmid:25569250; PubMed Central PMCID: PMC4287532.
Kho S, Qotrunnada L, Leonardo L, Andries B, Wardani P, Fricot A, et al. Evaluation of splenic accumulation and colocalization of immature reticulocytes and Plasmodium vivax in asymptomatic malaria: A prospective human splenectomy study. PLoS Med. 2021.
Seydel KB, Kampondeni SD, Valim C, Potchen MJ, Milner DA, Muwalo FW, et al. Brain swelling and death in children with cerebral malaria. N Engl J Med. 2015;372(12):1126–37. Epub 2015/03/19. pmid:25785970; PubMed Central PMCID: PMC4450675.
Laothamatas J, Sammet CL, Golay X, Van Cauteren M, Lekprasert V, Tangpukdee N, et al. Transient lesion in the splenium of the corpus callosum in acute uncomplicated falciparum malaria. Am J Trop Med Hyg. 2014;90(6):1117–23. Epub 2014/03/13. pmid:24615139; PubMed Central PMCID: PMC4047739.
Frolich AM, Tober-Lau P, Schonfeld M, Brehm TT, Kurth F, Vinnemeier CD, et al. Brain magnetic resonance imaging in imported malaria. Malar J. 2019;18(1):74. pmid:30871543 Central PMCID: PMC6419340.
Sugiyama M, Ikeda E, Kawai S, Higuchi T, Zhang H, Khan N, et al. Cerebral metabolic reduction in severe malaria: fluorodeoxyglucose-positron emission tomography imaging in a primate model of severe human malaria with cerebral involvement. Am J Trop Med Hyg. 2004;71(5):542–5. pmid:15569780.
Kawai S, Ikeda E, Sugiyama M, Matsumoto J, Higuchi T, Zhang H, et al. Enhancement of splenic glucose metabolism during acute malarial infection: correlation of findings of FDG-PET imaging with pathological changes in a primate model of severe human malaria. Am J Trop Med Hyg. 2006;74(3):353–60. pmid:16525091.
Jeph S, Thakur K, Shamim S, Aggarwal A. Malaria masquerading as relapse of Hodgkin’s lymphoma on contrast enhanced 18 F-fluorodeoxyglucose positron emission tomography/computed tomography: A diagnostic dilemma. Indian J Nucl Med. 2014;29:102–4. pmid:24761064
Rockett RJ, Tozer SJ, Peatey C, Bialasiewicz S, Whiley DM, Nissen MD, et al. A real-time, quantitative PCR method using hydrolysis probes for the monitoring of Plasmodium falciparum load in experimentally infected human volunteers. Malar J. 2011;10:48. pmid:21352599; PubMed Central PMCID: PMC3055851.
McCarthy JS, Sekuloski S, Griffin PM, Elliott S, Douglas N, Peatey C, et al. A pilot randomised trial of induced blood-stage Plasmodium falciparum infections in healthy volunteers for testing efficacy of new antimalarial drugs. PLoS ONE. 2011;6(8):e21914. pmid:21887214
Griffin P, Pasay C, Elliott S, Sekuloski S, Sikulu M, Hugo L, et al. Safety and Reproducibility of a Clinical Trial System Using Induced Blood Stage Plasmodium vivax Infection and Its Potential as a Model to Evaluate Malaria Transmission. PLoS Negl Trop Dis. 2016;10(12):e0005139. pmid:27930652; PubMed Central PMCID: PMC5145139.
Karunanithi S, Soundararajan R, Sharma P, Naswa N, Bal C, Kumar R. Spectrum of Physiologic and Pathologic Skeletal Muscle (18)F-FDG Uptake on PET/CT. AJR Am J Roentgenol. 2015;205(2):W141–9. pmid:26001118.
Kumar P, Patel CD, Singla S, Malhotra A. Effect of duration of fasting and diet on the myocardial uptake of F-18-2-fluoro-2-deoxyglucose (F-18 FDG) at rest. Indian J Nucl Med. 2014;29(3):140–5. Epub 2014/09/12. pmid:25210278; PubMed Central PMCID: PMC4157186.
Lodge MA. Repeatability of SUV in Oncologic (18)F-FDG PET. J Nucl Med. 2017;58(4):523–32. pmid:28232605; PubMed Central PMCID: PMC5373499.
Paquet N, Albert A, Foidart J, Hustinx R. Within-patient variability of (18)F-FDG: standardized uptake values in normal tissues. J Nucl Med. 2004;45(5):784–8. Epub 2004/05/12. pmid:15136627.
Gheysens O, Postnov A, Deroose CM, Vandermeulen C, de Hoon J, Declercq R, et al. Quantification, Variability, and Reproducibility of Basal Skeletal Muscle Glucose Uptake in Healthy Humans Using 18F-FDG PET/CT. J Nucl Med. 2015;56(10):1520–6. Epub 2015/08/01. pmid:26229142.
Gaur AH, McCarthy JS, Panetta JC, Dallas RH, Woodford J, Tang L, et al. Safety, tolerability, pharmacokinetics, and antimalarial efficacy of a novel Plasmodium falciparum ATP4 inhibitor SJ733: a first-in-human and induced blood-stage malaria phase 1a/b trial. Lancet Infect Dis. 2020. pmid:32275867.
Collins KA, Wang CY, Adams M, Mitchell H, Robinson GJ, Rampton M, et al. A Plasmodium vivax experimental human infection model for evaluating efficacy of interventions. J Clin Invest. 2020. pmid:32045385.
Roth E Jr., Plasmodium falciparum carbohydrate metabolism: a connection between host cell and parasite. Blood Cells. 1990;16(2–3):453–60; discussion 61–6. Epub 1990/01/01. pmid:2257322.
Shivapurkar R, Hingamire T, Kulkarni AS, Rajamohanan PR, Reddy DS, Shanmugam D. Evaluating antimalarial efficacy by tracking glycolysis in Plasmodium falciparum using NMR spectroscopy. Sci Rep. 2018;8(1):18076. pmid:30584241; PubMed Central PMCID: PMC6305384.
Heuker M, Sijbesma JWA, Aguilar Suarez R, de Jong JR, Boersma HH, Luurtsema G, et al. In vitro imaging of bacteria using (18)F-fluorodeoxyglucose micro positron emission tomography. Sci Rep. 2017;7(1):4973. pmid:28694519; PubMed Central PMCID: PMC5504029.
Adams WL. The role of the spleen in infectious diseases. Pac Med J. 1897;40(227).
Lubitz JM. Pathology of rupture of the spleen in acute vivax malaria. Am J Pathol. 1948;24(3):724. pmid:18859406; PubMed Central PMCID: PMC1942795.
Imbert P, Rapp C, Buffet PA. Pathological rupture of the spleen in malaria: analysis of 55 cases (1958–2008). Travel Med Infect Dis. 2009;7(3):147–59. Epub 2009/05/05. pmid:19411041.
Safeukui I, Correas JM, Brousse V, Hirt D, Deplaine G, Mule S, et al. Retention of Plasmodium falciparum ring-infected erythrocytes in the slow, open microcirculation of the human spleen. Blood. 2008;112(6):2520–8. Epub 2008/06/27. pmid:18579796.
Buffet PA, Safeukui I, Milon G, Mercereau-Puijalon O, David PH. Retention of erythrocytes in the spleen: a double-edged process in human malaria. Curr Opin Hematol. 2009;16(3):157–64. pmid:19384231.
Fernandez-Becerra C, Bernabeu M, Castellanos A, Correa BR, Obadia T, Ramirez M, et al. Plasmodium vivax spleen-dependent genes encode antigens associated with cytoadhesion and clinical protection. Proc Natl Acad Sci U S A. 2020;117(23):13056–65. pmid:32439708
Joice R, Nilsson SK, Montgomery J, Dankwa S, Egan E, Morahan B, et al. Plasmodium falciparum transmission stages accumulate in the human bone marrow. Sci Transl Med. 2014;6(244):244re5. pmid:25009232; PubMed Central PMCID: PMC4175394.
Brito MAM, Baro B, Raiol TC, Ayllon-Hermida A, Safe IP, Deroost K, et al. Morphological and Transcriptional Changes in Human Bone Marrow During Natural Plasmodium vivax Malaria Infections. J Infect Dis. 2020. pmid:32556188.
Odedra A, Webb L, Marquart L, Britton L, Chalon S, Moehrle J, et al. Liver function test abnormalities in experimental and clinical Plasmodium vivax infection. Am J Trop Med Hyg. 2020;103(5):1910–7. pmid:32815508; PubMed Central PMCID: PMC7646782.
Chughlay FM, Akakpo S, Odedra A, Csermak-Renner K, Djeriou E, Winnips C, et al. Liver enzyme elevations in Plasmodium falciparum volunteer infection studies: findings and recommendations. Am J Trop Med Hyg. 2020;103(1):378–93. Epub 20 April 2020. PubMed Central PMCID: PMC7356411. pmid:32314694
Woodford J, Shanks GD, Griffin P, Chalon S, McCarthy JS. The Dynamics of Liver Function Test Abnormalities after Malaria Infection: A Retrospective Observational Study. Am J Trop Med Hyg. 2018;98(4):1113–9. pmid:29436349; PubMed Central PMCID: PMC5928828.
Douglas NM, Anstey NM, Buffet PA, Poespoprodjo JR, Yeo TW, White NJ, et al. The anaemia of Plasmodium vivax malaria. Malar J. 2012;11:135. pmid:22540175; PubMed Central PMCID: PMC3438072.
Kho S, Barber BE, Johar E, Andries B, Poespoprodjo JR, Kenangalem E, et al. Platelets kill circulating parasites of all major Plasmodium species in human malaria. Blood. 2018;132(12):1332–44. pmid:30026183
Woodford J, Yeo TW, Piera KA, Butler K, Weinberg JB, McCarthy JS, et al. Early Endothelial Activation Precedes Glycocalyx Degradation and Microvascular Dysfunction in Experimentally Induced Plasmodium falciparum and Plasmodium vivax Infection. Infect Immun. 2020;88(5). pmid:32122938; PubMed Central PMCID: PMC7171246.
de Mast Q, Groot E, Lenting PJ, de Groot PG, McCall M, Sauerwein RW, et al. Thrombocytopenia and release of activated von Willebrand Factor during early Plasmodium falciparum malaria. J Infect Dis. 2007;196(4):622–8. pmid:17624850.
Karanikas G, Zedwitz-Liebenstein K, Eidherr H, Schuetz M, Sauerman R, Dudczak R, et al. Platelet kinetics and scintigraphic imaging in thrombocytopenic malaria patients. Thromb Haemost. 2004;91(3):553–7. Epub 2004/02/26. pmid:14983232.