- Open Access
Comparative pharmacokinetics and pharmacodynamics of intravenous artelinate versus artesunate in uncomplicated Plasmodium coatneyi-infected rhesus monkey model
© The Author(s) 2016
Received: 5 April 2016
Accepted: 28 July 2016
Published: 6 September 2016
The US Army designed artelinate/lysine salt (AL) to overcome the instability of sodium artesunate in aqueous solution (AS). To select the most efficacious artemisinin treatment, direct comparison was performed in an uncomplicated non-human primate malaria model.
Splenectomized rhesus monkeys were inoculated with Plasmodium coatneyi and on day six, single equimolar loading dose of IV AL (11.8 mg kg−1) or IV AS (8 mg kg−1) were administered followed by 1/2 the first dose once daily for 2 more days. Blood smear were performed twice daily and the number of parasites were counted microscopically. Blood samples were obtained after the first dose within 6 h for pharmacokinetic (PK) and ex vivo pharmacodynamic evaluation by simultaneously measuring plasma drug concentration and anti-malarial activity against Plasmodium falciparum in vitro.
The anti-P. coatneyi in vivo activity of both compounds were comparable, but the ex vivo anti-P. falciparum potency of the IV AS regimen as administered was sevenfold higher than that of IV AL. Comparing in vivo pharmacodynamics of AL and AS, daily assessed parasite counts showed comparable 99 % parasite clearance times (PC99: 2.03, 1.84 day), parasite clearance rates (5.34, 4.13 per min) and clearance half-life (PCt1/2: 7.79, 10.1 h). This study showed strong and significant inverse correlation between PCt1/2 and t1/2 of AS + DHA, and AUC0–∞ of DHA, and correlated with Vz of AS (r2 > 0.7, p ≤ 0.002). Lastly, following IV AL, there was a modest inverse correlation between PCt1/2 and Cmax (r2 0.6, p ≤ 0.04). Although all tested monkeys recrudesced subsequently, two died following AL regimen before parasite clearance. While the aetiology of those deaths could not be definitively determined, pathologic evidence favoured a sepsis-like syndrome and suggested that severe malaria was more likely than drug toxicity.
The model demonstrated that both AS and DHA contributed to the anti-malarial activity of IV AS, while IV AL activity was largely restricted to the parent drug. Parasite clearance was strongly and linearly dependent on drug exposure for both artemisinin regimens. However, IV AS had higher ex vivo potency against P. falciparum, leading to an IND filing for GMP manufactured AS in the United States.
Despite reductions in morbidity and mortality, severe malaria still kills a half a million persons worldwide each year, including travelers . Severe malaria occurs when Plasmodium infection is complicated by serious organ failure or metabolic abnormalities which develop rapidly and can progress to death within 24–48 h, and requires parenteral therapy. Since 1991, quinidine gluconate remains the only FDA-approved drug available for severe malaria infection in the US. It is available in limited supply, requires continuous infusion with a loading dose in an intensive care unit for cardiac and glycaemic monitoring, and resistance has been documented [2, 3]. Artesunate (AS) was developed and tested as a replacement for quinine. AS has now been receiving WHO-prequalification status since 2010 and adopted as the recommended treatment; but a Good Manufacture Practice (GMP) product remains inaccessible in many countries . Intravenous AS was associated with a lower risk of hypoglycaemia and has been shown to significantly reduce the risk of death from severe malaria compared to IV quinine [5, 6]. Artesunate is also a more practical option in resource-poor settings since administration is simpler (by bolus injection) and does not require slow rate-controlled infusion as well as cardiac monitoring [5, 7].
During the testing of parenteral artesunate, the US Army, through the Walter Reed Army Institute of Research, had considered developing another artemisinin derivative, artelinic acid-l-lysine salts (AL) and was patented in 1988  as anti-malarial agents for clinical treatment of severe malaria. Artelinate, a semi-synthetic derivative of artemisinin, does not convert readily to dihydroartemisinin (DHA) was designed to overcome the instability of sodium artesunate in aqueous solution, which must be prepared at the bed side before injection. Pre-clinical efficacy and toxicity studies were used to select one of these artemisinin candidates as potential treatments for severe malaria and eventual FDA registration. Comparative anti-malarial efficacy of IV AL and AS in rat malaria model showed that AL had a superior anti-malarial potency than AS in terms of parasitaemia clearance . However, this evidence also showed that AL was more toxic than AS in rats [10, 11].
Several non-human primate malaria models serve as useful surrogates to evaluate new drugs prior to testing in humans. Plasmodium coatneyi is primate malaria that causes tertian malaria in splenectomized Asian macaques, complicated by sequestration of the infected erythrocytes and a high mortality rate in untreated animals . This model most closely mimics severe and complicated malaria caused by Plasmodium falciparum [13, 14]. Limited efforts have used this model to study toxicity of drug due to brain-damage induced by lipid-soluble depot artemisinins [13, 15]. The present study compared the pharmacokinetics and pharmacodynamics of AL and AS in the uncomplicated P. coatneyi infected rhesus monkey model to test the new candidate drugs for severe malaria treatment.
The United States Army Medical Component, Armed Forces Research Institute of Medical Sciences (USAMC-AFRIMS) Institutional Animal care and Use Committee and the Animal Use Review Division, US Army Medical Research and Materiel Command reviewed and approved the protocol. Research was conducted in 2002 in compliance with the Animal Welfare Act and other federal statutes and regulations relating to animals and experiments involving animals and adheres to principles stated in the Guide for the Care and Use of Laboratory Animals, NRC Publication, 1996 edition. The USAMC-AFRIMS animal care and use programme has been accredited by Association for Assessment and Accreditation for Laboratory Animal Care International since 1999.
Plasmodium coatneyi-Rhesus monkey model
Plasmodium coatneyi-infected RBCs (wild-type strain originally donated by W.E. Collins, CDC, Atlanta, GA) were maintained as cryopreserved stabilates at AFRIMS, Bangkok, Thailand. The stabilate stock was tested and confirmed negative for B-virus, SRV, SIV and STV-1 to ensure no adventitious viruses transmission were introduced to the monkey colony. Twenty-two adult colony-born, Indian-origin rhesus macaques (Macaca mulatta) naïve monkeys were splenectomized and recovered well more than 1 month prior to entering the study. All monkeys were free from B-virus, SIV, SRV and STLV antibodies. Animal health screening included complete physical examination, CBC, ALT and creatinine. Twenty-two animals were randomized to two experiments of 11 monkeys. Each experiment included ten experimental monkeys (IV AL and AS) and one control animal. The control monkeys received intramuscular quinine treatment and the experimental animals received intravenous artemisinin candidates.
Infected donor monkey
For each experiment, after thawing a stabilate of P. coatneyi-infected erythrocytes, 1 ml aliquot was inoculated intravenously to the test monkey. The monkey was sedated with ketamine HCl (5–15 mg kg−1, IM) for this procedure. Parasitaemia levels were monitored daily. After the parasite density reached >50,000 parasites µl−1, 5–20 ml of blood was drawn from a femoral vein into a heparinized tube. Blood was divided into 1 ml aliquots (about 5 × 106 RBC with a 1 % parasitaemia) for inoculation of the study animals. Then, the donor animal was treated with chloroquine hydrochloride 10 mg kg−1 day−1 IM for 5–7 days. This was the standard treatment regimen for P. coatneyi-infected control animals at AFRIMS based on local protocols. The injectable chloroquine hydrochloride (Aralen™ 40 mg base/ml) was given by intramuscular route. The injection has been practical since it can be given with minimal animal handling using the “squeeze cage” mechanism. Animals were monitored daily and the treatment range of 5–7 days was used as the benchmark for when blood smear evaluation became negative.
Parasitaemia and clinical monitoring
Animals were observed at least twice daily to assess clinical signs and correlates of severe malaria. Based on our previous model validation, blood smears were performed to detect malaria parasites starting prior to inoculation on day 0 and continued daily (0700–0800 h). The monkeys were physically restrained in the squeeze cage restraint apparatus and approximately 0.1–0.2 ml whole blood was collected from each monkey by lancet puncture of the lateral auricular vein. Thick and thin smears were made on the same microscope glass slide and subsequently fixed in methanol and stained with Giemsa. When the smears were positive, white blood cell count (WBC) and/or red blood cell count (RBC) were also performed using automated haematology analyzer Sysmex K800 to calculate parasite density. Haematocrits were checked as needed. At study days 6–12, additional blood samples were obtained from all animals in the afternoon (1500–1600 h) to monitor parasitaemia levels. Daily blood smears were continued until two consecutive days with negative smears. Then the smear monitoring schedule was reduced to two times weekly for 2 weeks and then weekly for 6 weeks after completion of the last treatment. Treatment failures and/or recrudescence were treated with IM quinine dihydrochloride 60 mg kg−1 loading dose, followed by 30 mg kg−1, every 8 h for 3 days.
Treatment was initiated at parasitaemias ≥3 % or >200,000 parasites µl−1 (on study day 6 morning) due to rapid increasing in parasitaemia levels observed in previous model development and dose-ranging studies (unpublished data). Blood smear staining and parasitaemia determination took about 2 h. The first dose of treatment was decided after the results were confirmed. The eleven monkeys were treated as one cohort when the majority met the treatment criteria and allowed for practical blood drawing and processing for PK sampling. The control monkey received quinine treatment and the ten experimental animals received intravenous artemisinin derivative candidate. Animals were pole-and-collar trained and sat in restraining chairs to receive the IV injection and phlebotomy without the use of chemical restraint to avoid potential confounding and depression by concomitant anesthetic administration.
Artelinic acid (WR255663), 4-(10′ dihyro-artemisinin-oxymethyl) benzoic acid hemihydrate, was prepared as an l-lysine salt (MW 573.719) powder at Walter Reed Army Institute of Research (WRAIR; Silver Springs, MD) and shipped to AFRIMS through WRAIR Chemical Information. Artesunic acid (MW 384.425) and 5 % sodium bicarbonate solution was obtained from Guilin Pharmaceutical, Guangxi, China and imported by Atlantic Pharmaceutical Co., Ltd., Bangkok, Thailand. Artelinate/lysine salt (AL) powder prepared with 1 g of the acid content was equivalent to 1.35 g of the salt weight. Intravenous AL was prepared from a stock solution containing 40 mg L−1 of AL by dissolving the calculated amount of the AL salt in a solution of 0.45 % NaCl/0.1 % l-lysine (w/v), sterilized and filtered through 0.2 µm cellulose acetate. Additional IV solutions with the required concentrations of AL was made by appropriate dilution of the 40 mg L−1 solution with normal (0.9 %) saline containing 0.1 % l-lysine, followed by filtration through a syringe filter prior to use. Intravenous artesunate/sodium salt (AS) was prepared by dissolving the acid in 5 % sodium bicarbonate just prior to injection per manufacturer instructions.
Single, equimolar doses 20 μmol of IV AL (11.8 mg kg−1) and IV AS (8 mg kg−1) were administered as a rapid bolus injection over a 1-min period. These doses were chosen as the minimal effective doses (from previous model development and validation studies, unpublished data) and blood was collected for pharmacokinetic analysis. After a week wash-out and recovery period, P. coatneyi (1 mL of >50,000 parasitized RBCs per microlitre or 5 × 106 RBC with a 1 % parasitaemia) were inoculated from a donor monkey into all the monkeys. The treatment was initiated at day 6 after inoculation at a parasitaemia ≥3 % or >200,000 parasites μL−1 when the cohort of animals was minimally symptomatic. Drugs were given for 3 days with a loading dose initially followed by ½ of the first dose on the 2nd and 3rd days. Consequently, each monkey served as its own control for intra-subject variation, and differences are likely due to the disease effects from malaria infection.
Blood collection and sample preparation
Blood was collected for pharmacokinetic/pharmacodynamics (PK/PD) analysis after the first dose only due to rapid clearance of artemisinin derivatives. Heparinized blood was collected at 0, 5, 20, 40 min, 1, 3, and 6 h post-dose and plasma samples were separated within 2 h by centrifugation (1500g, 10 min). Aliquots of samples were made for simultaneous measurement by HPLC  and bioassay , and stored at −80 °C until analysis. All glassware was silanized before use with a 0.5 % aqueous solution (v/v) of Pierce Aquasil (Rockford, IL, USA) according to the manufacturer’s recommended procedure. Solid-phase extraction was performed on C-18 elution cartridge (3.0 ml, J.T. Baker Co.) using a VAC ELUTE SPS24 sample processing station (Analytichem International, Harbour City, CA, USA). The cartridge was preconditioned by sequential washing with 2.5 ml acetonitrile, 2.5 ml methanol and 2.5 ml water. One ml of distilled water was added to the cartridge before adding plasma sample (0.5 ml). Then, the cartridge was washed with 2.5 ml distilled water, 2.5 ml of 0.05 % H3PO4 (pH 4.5) and 2.5 ml of 20 % acetonitrile and completely dried by closing the vacuum for 15 min. The analytes were collected by eluting with 0.5 ml methanol three times and then with 0.5 ml 90:10 n-butyl chloride: ethyl acetate twice. The organic phases were pooled. The combined organic phases were then evaporated to dryness under a stream of nitrogen at room temperature. Extraction residues were reconstituted with 50:50 ethanol: water (0.3 ml), at least 16 h before injection. The injection volume was 100 µl for all samples.
The plasma concentration of parent drugs, AL and AS, and their primary metabolites, DHA and 2-hydroxyartelinate (OHAL) respectively, were measured by HPLC with electrochemical detection in reductive mode (HPLC-ECD) , which was the only method for artemisinin compounds then (Additional files 1 and 2). The total anti-malarial activity of the drug and all active metabolite(s) in plasma were measured by bioassay against in vitro P. falciparum clone (W2) and expressed as DHA equivalents  (Additional file 3).
HPLC with reductive electrochemical detection was performed using a model BAS 200B liquid chromatography (Bioanalytical Systems, Inc., West Lafayette, Indiana, USA). A Nova-Pak® C18 (3.9 × 150 mm, Waters Corporation, Milford, MA, USA) was used with 40 % acetonitrile in sodium acetate buffer (pH 3.6) as mobile phase. Detection was performed using a thin dual-layer glassy carbon electrode run in parallel mode at a potential of −1.0 V versus Ag/AgCl. The system was operated at the following temperatures: mobile phase 35 °C, column and detector oven 30 °C, cell 31 °C with the flow rate of 1.5 mL min−1. Artemisinin (ART) was used as an internal standard. Samples were injected via Gilson model 231 XL sampling injector equipped with a 100 µL loop, a Gilson model 401 dilutor/pipettor, a sampler controller keypad (Gilson Medical Electronics, Middleton, WI, USA), and a Valco electrically actuated switching valve (Valco Instrument Co. Inc) was used. This system automatically deoxygenated and injected sample, which permits the high sample throughput associated with automated injection. Data were acquired and analysed using a Millennium32 Chromatography Manager (Waters Corporation, Milford, MA, USA).
Standard curve and quality control samples were prepared by spiking plasma with 50:50 ethanol:water solutions of AS with DHA or AL with OHAL. The final concentration range was from 10 to 2000 ng mL−1 plasma. Artemisinin 250 ng mL−1 was added as an internal standard to all samples.
Ex vivo Plasmodium falciparum-based bioassay (BA)
The plasma anti-malarial activities of the artemisinin derivatives were measured using a previously published method . In brief, plasma was incubated with protein A to remove the majority of immunoglobulin (IgG) that results in the lysis of the parasites in the erythrocytes (heat treatment was not used due to the effect on the stability of artemisinin derivatives in plasma). After centrifugation, the supernatant (100 µL) was transferred to a 96-well flat bottom plate. Twofold serial dilutions were then made using heat inactivated pooled control serum (human:rhesus = 1:1). A suspension of malaria (W2 clone) infected erythrocytes was added to each well. The microtitre plate was placed into a gas-tight plexiglass chamber, flushed with a gas mixture of 90 % CO2, 5 % O2, and 5 % N2, and placed into an incubator (37 °C). Following 24 h incubation, the plate was removed from the chamber and pulsed with [3H]-hypoxanthine solution to each well and incubated for another 18–20 h before harvesting. The incorporation of [3H]-hypoxanthine by the parasites in each well was determined by counting in a scintillation counter.
A dose–response curve for each plasma sample was constructed by plotting [3H]-hypoxanthine uptake on the Y-axis against the corresponding dilution factor on the X-axis after logarithmic transformation. The dilution factor value that inhibits parasite growth by 50 % (DF50) of each plasma sample was determined. Using the DF50 value, the anti-malarial activity of the plasma sample was extrapolated from a linear standard curve using DHA, the most potent artemisinin derivative, and expressed as DHA equivalents.
Assessment of parasite counts
Blood smear were collected once daily in the morning. Once positive parasitaemia was observed and reached 2000 parasites μL−1, blood smears were collected twice, in the morning and afternoon. Blood for slides preparation were collected from ear for thick and thin smear preparation. Blood films on glass slides were air dried, fixed with 100 % methanol, stained with Giemsa, and read under ×100 magnification oil emersion for parasite determination.
Blood CBC was determined by automated haematology analyzer Sysmex K800 every other day. When parasite density was greater than ten parasites/field, parasites were counted per 1000 RBC. Thin smear was used when number of parasite was greater than five parasites per field in thick film. For counting parasite density/RBC, a grid micrometre was used and the number of parasitized RBCs was used for calculation. If the parasite density was less than ten parasites μL−1 the determination of parasitaemia was counted per 100 WBC (calculation method of parasite number was the same as thick smear).
The number of asexual parasites μL−1 of whole blood was determined by counting white blood cells (WBC) in high-power fields containing a total of 500 parasites if the ratio of parasites/WBC was more than one, or the number of parasites per 1000 WBCs was counted if the ratio of parasites/WBC was less than one. The parasitaemia level was calculated as the product of the parasite/WBC ratio and the WBC count (microscope filed that is well-populated with WBCs (20 WBCs/field) and five views were used for parasitaemia count).
In vivo pharmacodynamics (iPD) analysis
The parasite density-time curve was constructed and the parasite clearance parameters were estimated using Parasite Clearance Estimator . The parameters were parasite clearance rate (PCR), clearance half-life (PCt½), PC50, PC95, PC99 (PCn—defined as the time from initiation of treatment to the time parasites were cleared by n %). In addition, the parasite clearance time (PCT) by conventional method (defined as the time from initiation of treatment to the time the first two consecutive negative blood smears) was assessed by microscopy.
Non-compartmental analysis was used to derive pharmacokinetic parameters of AS and its metabolite DHA, AL and its metabolite OHAL, using WinNonlin™ Standard Edition, v 2.1 (Pharsight Corporation, Cary, NC, USA). The PK parameters determined were the elimination rate constant (λz) was calculated by least-squares regression analysis of the ln-linear portion of the plasma concentration–time curve (the number of time points >3). The elimination half-life (t1/2) was calculated from the ratio of 0.693/λz, the maximum concentration (Cmax) in plasma and the time to reach Cmax after dosing (Tmax) were obtained by inspection, the area under the concentration–time curve (from time zero to 20 min, AUC0–20, and zero to infinity, AUC0–∞) was estimated by the linear trapezoidal rule. The apparent total body clearance (Cl) and volume of distribution (Vz) associated with the terminal phase were calculated as dose/AUC, and Cl/λz, respectively.
Statistical comparison between dosage regimens was performed using the Mann–Whitney U test and all the values reported were in median with 25th and 75th interquartile. The correlation between two variables was performed using simple linear regression model with least square method. Results were considered statistically significant when the p value was <0.05. (Prism 6 for Windows v. 6.01)
Clinical results and in vivo pharmacodynamics (iPD)
The initial status of the monkeys and in vivo pharmacodynamics, parasites clearance values
Parasites clearance rate (PCR)
Parasites clearance half-life (PCt1/2)
95 % Parasites clearance (PC95)
99 % Parasites clearance (PC99)
Parasites clearance (PCT)c
Pharmacokinetics of intravenous artelinate and artesunate in plasma from P. coatneyi infected rhesus monkeys
Parent compound (P)
C max b
t 1/2 c
AUC 0–∞ d
AUC 0–20 e
L kg−1 min−1
V z g
Ex vivo pharmacodynamic (ePD)
Pharmacokinetic parameters based on combined parent drug and metabolite levels and ex vivo pharmacodynamics (ePD)
Ex vivo pharmacodynamica
Combined P + M
Ex vivo potency
C max c
t 1/2 d
AUC 0–∞ e
AUC 0–20 f
L kg−1 min−1
V z h
Figure 3 indicated that the anti-malarial activity of IV AS was contributed by both the parent drug AS and its active metabolite DHA until 20 min post-dose when the major compound in plasma transitioned to DHA. Parent drug AS was below the detection limit beyond 1 h post-dose and DHA was detected at its highest level as early as 5 min post-dose. As a result, AUC0–20 was 97 % of AUC0–∞ for AS and 53 % for combined AS + DHA (Tables 2, 3). On the other hand, although OHAL metabolite was detected by HPLC-ECD, only AL was responsible for plasma anti-malarial activity (Fig. 3) and the AUC0–20 compared to the corresponding AUC0–∞ for AL and AL + OHAL which were comparable at 24.6 and 21.4 % respectively (Tables 2, 3). Furthermore, no DHA was found in plasma from either healthy or infected monkeys treated with IV AL.
Based on testing against the W2 clone, the in vitro potency of AS was comparable to DHA and was 4–5 times greater than that of AL. Since AS and its metabolite DHA contributed to the plasma anti-malarial activity, ex vivo potency was then determined from the AUC0–∞ ratio between ePD and PK of the combined parent and its metabolite (Table 3). Thus, the ex vivo potency of IV AS (0.643) was sevenfold greater than IV AL (0.088).
Pharmacokinetic/pharmacodynamic correlation analysis (least square regression)
Correlation between PK and ePD
PK-ePD linear regression
AUC0–∞ (mM min)
AUC0–20 (mM min)
PK or ePD)/iPD
Linear regression analyses between PK or ePD and iPD
L kg−1 min−1
AS + DHA
L kg−1 min−1
AUC 0 –∞
While direct comparison of safety and efficacy were complicated by experimental factors, IV AS proved to have superior potency and more rapid parasite clearance compared to IV AL. Similar to prior studies in humans [15, 18, 19], PK/PD relationships for AS in monkeys revealed that the parent drug AS was rapidly converted to DHA and undetectable as early as 1 h post-dose. Activity and metabolic conversion were rapid. While AS was at fourfold higher concentration at 5 min post dose, only DHA remained responsible for the observed anti-malarial activity roughly 20 min post-dose when plasma concentrations of DHA far exceeded AS. The t1/2 of DHA was at least ninefold longer than AS. This is consistent with prior observations in healthy human studies attributing the effectiveness of AS in part to its rapid and extensive hydrolysis to DHA, achieving high initial drug levels .
Challenges inherent to the model limit experimental interpretation to some degree. The two experimental groups were inoculated and dosed separately rather than concurrently to allow sufficient time to adequately perform all procedures. Based on previous model development, the number of P. coatneyi parasites was expected to increase rapidly on study day 6. Therefore, blood parasitaemia was not measured prior to treatment in order to limit overall blood draws. Animals in the IV AS group were dosed first and morning parasitaemia levels varied between 0.5 and 10.1 %, while parasitaemia in IV AL animals was between 7.1 and 20.2 %, with roughly twofold higher median parasitaemia in the IV AL group (12 %) compared to IV AS (6.6 %) at initial dose. To some extent, this makes a meaningful in vivo PK/PD comparison difficult. Moreover, there were two deaths in the IV AL group limiting available data from those animals. Baseline parasitaemias in these animals (13.2 and 13.0 %) were comparable to those of other animals. Both monkeys died when their parasite density reached 1.2 × 106 parasites μL−1. Parasitaemias were 15 and 20 % respectively at 1 h apart suggesting that malaria was at the very least a major contributor to their demise. Although the aetiology of death could not be determined definitively, pathologic examination favored a systemic inflammatory syndrome consistent with severe malaria over drug toxicity.
The P. coatneyi model requires splenectomy in order to ensure adequate parasite infection and determine efficacy, and the results should be interpreted in light of this consideration. Normally, the spleen removes abnormal erythrocytes and intra-erythrocytic inclusions, including dead parasites which are removed from erythrocytes without erythrocyte destruction by the spleen . Infected RBCs may persist longer and likely delayed parasite clearance compared to what would have been observed in spleen-intact animals. In a tissue distribution study in rats, 1 h following IV administration of AS, high levels of AS were found in brain, fat, intestine and serum, with comparatively low levels in other tissues including liver, kidney, testicle, muscle, fat, heart, eye, spleen and lung . Splenectomy was unlikely to have had a significant effect on the PK parameters and metabolism of AS or AL given the short half-life of both drugs.
In light of these findings, the human-rhesus dose conversion factor can be derived based on PK parameters.
The ePD of IV AS in uncomplicated P. coatneyi-infected rhesus monkey (8 mg kg−1 dose) can be directly compared to that of patients with uncomplicated falciparum malaria (2 mg kg−1 dose) . Using total drug exposure, AUC values in human vs rhesus (636 vs 476 µM min), the AUC per unit dose for human was 318 and that of rhesus was 59.5. Therefore, the approximate inter-species conversion factor for human in relation to rhesus is 5.34.
From Eq. (2), if the human dose = 2 mg kg−1,
Rhesus equivalent dose = 5.34*2
=10.7 mg kg−1
Vice versa, if the Rhesus dose = 8 mg kg−1,
Human equivalent dose = 8/5.34
Cmax, µmol L−1
AUC, µmol min L−1
Cl, L h−1 kg−1
Vd, L kg−1
AUC, µmol min L−1
Dose, mg kg−1
Studies in multiple species [23, 24] have demonstrated limited conversion of AL to DHA. However, we found no DHA in rhesus plasma at all, instead detecting the OHAL metabolite by HPLC-ECD in accordance with a previous report suggesting that this is a product of rhesus monkey microsomes . This finding indicates that the parent drug AL alone contributed to blood stage anti-malarial activity, and is concordant with earlier work also demonstrating in vitro conversion of AL into OHAL in human liver microsomes [25, 26]. Furthermore, the effect of IV AS and IV AL on P. coatneyi recrudescence seen here in non-human primates was similar to that seen for Plasmodium vinckei in rodents , suggesting the possibility that both AS and AL may trigger in vivo parasites dormancy in NHPs. This has been postulated as an underlying mechanism of treatment failure for artemisinin monotherapy . Nevertheless, recrudescence due to short-course artemisinin treatment can be overcome by the use of combination therapy with slow acting anti-malarial agents .
Correlation between drug exposure (PK) and drug effect (PD) for artemisinin compounds has been challenging due to rapid clearance of drug, unclear mechanism of action, and sequestration in red blood cells combined with the inability to measure intraerythrocytic drug levels. Parasite clearance, a function of host-parasite-drug interactions, is a good measure of the in vivo drug effect. Davis et al.  reported only a borderline significant inverse correlation between AUC and PC50 following IV AS therapy for severe malaria in a 2001 study. Ten years later, White  demonstrated that the parasite clearance time was associated with parasite density, potentially confounding PK/PD correlations with artemisinins, and this was borne out in subsequent field studies of oral artesunate monotherapy . Bakshi et al.  developed a PK/PD in vitro system and found that the efficacy of artemisinin depended on Cmax while that of chloroquine depended on its time above minimum inhibitory concentration, TMIC, which were confirmed in an in vivo Plasmodium berghei-mouse model. Pooled analysis of data from severe malaria patients following IV AS revealed there was no significant association between PCt1/2 and post hoc population PK estimates. Lastly, children have been found to have lower DHA exposure than adults , with a recent study by Hawkes et al.  concluding that slower parasite clearance in children relative to adults may be explained by lower DHA exposure. However, they did not observe any correlation between DHA exposure and parasite clearance.
In present study using uncomplicated P. coatneyi-Rhesus monkey malaria model, PK-PD analysis of IV AS reveals an inverse linear correlation of DHA’s AUC with both PCt1/2 and PCT (Table 5) with longer PCt1/2 and PCT resulting from lower DHA exposure. This is consistent with Hawkes’ conclusion in humans suggesting that the rhesus model mimics human PK/PD for IV AS. Moreover, although AS is rapidly metabolized to DHA following IV administration, parasite clearance appears to be contributed by both components (Fig. 5) and the efficacy of IV AS depends on the t1/2 of combined AS + DHA > Vz of AS > AUC of DHA. In addition, IV AS had strong correlation between PK and iPD (in vivo drug effect against P. coatneyi-infected monkey) but not ePD (ex vivo drug effect against P. falciparum blood stage) and iPD suggesting that AS and DHA both contributed to in vivo activity against both blood and tissue parasite stages. On the other hand effect kinetic parameter Cmax for IV AL was inversely correlated with PCt1/2. The strong correlation between PK and ePD as well as ePD and iPD implied that the in vivo activity of AL may be predominantly blood stage activity.
In a non-human primate model of uncomplicated malaria, IV AS had greater ex vivo potency against P. falciparum with higher anti-P. falciparum activity during the first 20 min of drug administration. The model demonstrated that parasite clearance was dependent on drug exposure including both AUC and Cmax for both artemisinin regimens. While the efficacy of IV AS depended on the t1/2 of combined AS + DHA, the Vz of AS, and the AUC of DHA, efficacy of IV AL depended largely on its effect kinetic parameter Cmax, and was largely restricted to parent drug activity. As a result, IV AS was selected for further development for the treatment of severe malaria under an Investigational New Drug application (IND) held by the U.S. Army Office of the Surgeon General. In the United States, it is currently available to patients under an IND treatment protocol maintained at the Centers for Disease Control  and by the military.
PJW conceived and participated in the design of the study. RSM participated in the design and execution of the study. MG participated in the design, execution, and analyzed the data of the animal study. PT participated in the execution of the study, conducted the HPLC-ECD analysis and bioassay, performed data analysis, and drafted the manuscript. SK carried out the animal study. DS and NC carried out the HPLC-ECD analysis. MR and AL carried out the bioassay. DLS helped to draft the manuscript. All authors read and approved the final manuscript.
We are grateful to Dr. A.J. Lin from the Walter Reed Army Institute of Research for the synthesis of artelinic acid, the AFRIMS’ Department of Veterinary Medicine pre-clinical and laboratory teams for their technical support, husbandry of monkeys, and conducting microscopy. We are appreciative of our colleague at AFRIMS Somporn Krasaesub for advice on statistical analysis.
The authors declare that they have no competing interests.
This work was supported by Military Infectious Disease Research Program (MIDRP) “Drug to treat multi-drug resistant and severe and complicated malaria” under proposal MIDRP STO AQ00012_01_AF AND AQ00012_02_AF AQ0008_02_AF. Material has been reviewed by the Walter Reed Army Institute of Research. There is no objection to its presentation and/or publication. The opinions or assertions contained herein are the private views of the author, and are not to be construed as official, or as reflecting true views of the Department of the Army or the Department of Defense.
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- World Health Organization. World malaria report. Geneva: World Health Organization; 2015.Google Scholar
- Griffith KS, Lewis LS, Mali S, Parise ME. Treatment of malaria in the United States: a systematic review. JAMA. 2007;297:2264–77.View ArticlePubMedGoogle Scholar
- Chaijaroenkul W, Wisedpanichkij R, Na-Bangchang K. Monitoring of in vitro susceptibilities and molecular markers of resistance of Plasmodium falciparum isolates from Thai–Myanmar border to chloroquine, quinine, mefloquine and artesunate. Acta Trop. 2010;113:190–4.View ArticlePubMedGoogle Scholar
- Bartoloni A, Tomasoni L, Bartalesi F, Galli L, Sani S, Veloci S, et al. Combined intravenous treatment with artesunate and quinine for severe malaria in Italy. Am J Trop Med Hyg. 2010;83:274–6.View ArticlePubMedPubMed CentralGoogle Scholar
- Dondorp A, Nosten F, Stepniewska K, Day N, White N. South East Asian Quinine Artesunate Malaria Trial Group. Artesunate vs quinine for treatment of severe falciparum malaria: a randomised trial. Lancet. 2005;366:717–25.View ArticlePubMedGoogle Scholar
- Abdallah TM, Elmardi KA, Elhassan AH, Omer MB, Elhag MS, Desogi MA, et al. Comparison of artesunate and quinine in the treatment of severe Plasmodium falciparum malaria at Kassala hospital Sudan. J Infect Dev Ctries. 2014;8:611–5.View ArticlePubMedGoogle Scholar
- World Health Organization. Guidelines for the malaria treatment. WHO Guidelines Approved by the Guidelines Review Committee. Geneva: World Health Organization; 2015.Google Scholar
- Lin AJ, Klayman DL, Milhous WK. Novel water-soluble antimalarial dihydroartemisinin derivatives. U.S. Patent 4,791,135 1988. Dec 13.Google Scholar
- Li QG, Si YZ, Lee P, Wong E, Xie LH, Kyle DE, Dow GS. Efficacy comparison of intravenous artelinate and artesunate in Plasmodium berghei-infected Sprague–Dawley rats. Parasitology. 2003;126:283–91.View ArticlePubMedGoogle Scholar
- Li Q, Xie LH, Johnson TO, Si Y, Haeberle AS, Weina PJ. Toxicity evaluation of artesunate and artelinate in Plasmodium berghei-infected and uninfected rats. Trans R Soc Trop Med Hyg. 2007;101:104–12.View ArticlePubMedGoogle Scholar
- Xie LH, Johnson TO, Weina PJ, Si Y, Haeberle A, Upadhyay R, et al. Risk assessment and therapeutic indices of artesunate and artelinate in Plasmodium berghei-infected and uninfected rats. Int J Toxicol. 2005;24:251–64.View ArticlePubMedGoogle Scholar
- Smith CD, Brown AE, Nakazawa S, Fujioka H, Aikawa M. Multi-organ erythrocyte sequestration and ligand expression in rhesus monkeys infected with Plasmodium coatneyi malaria. Am J Trop Med Hyg. 1996;55:379–83.PubMedGoogle Scholar
- Maeno Y, Brown AE, Smith CD, Tegoshi T, Toyoshima T, Ockenhouse CF, et al. A nonhuman primate model for human cerebral malaria: effects of artesunate (qinghaosu derivative) on rhesus monkeys experimentally infected with Plasmodium coatneyi. Am J Trop Med Hyg. 1993;49:726–34.PubMedGoogle Scholar
- Teja-Isavadharm P, Peggins JO, Brewer TG, White NJ, Webster HK, Kyle DE. Plasmodium falciparum-based bioassay for measurement of artemisinin derivatives in plasma or serum. Antimicrob Agents Chemother. 2004;48:954–60.View ArticlePubMedPubMed CentralGoogle Scholar
- Newton PN, Barnes KI, Smith PJ, Evans AC, Chierakul W, Ruangveerayuth R, White NJ. The pharmacokinetics of intravenous artesunate in adults with severe falciparum malaria. Eur J Clin Pharmacol. 2006;62:1003–9.View ArticlePubMedGoogle Scholar
- Li QG, Peggins JO, Lin AJ, Masonic KJ, Trotman KM, Brewer TG. Pharmacology and toxicology of artelinic acid: preclinical investigations on pharmacokinetics, metabolism, protein and red blood cell binding, and acute and anorectic toxicities. Trans R Soc Trop Med Hyg. 1998;92:332–40.View ArticlePubMedGoogle Scholar
- Worldwide antimalarial resistance network. http://www.wwarn.org/toolkit/data-management/parasite-clearance-estimator. Accessed Apr 2015.
- Li Q, Cantilena LR, Leary KJ, Saviolakis GA, Miller RS, Melendez V, Weina PJ. Pharmacokinetic profiles of artesunate after single intravenous doses at 0.5, 1, 2, 4, and 8 mg/kg in healthy volunteers: a phase I study. Am J Trop Med Hyg. 2009;81:615–21.View ArticlePubMedGoogle Scholar
- Miller RS, Li Q, Cantilena LR, Leary KJ, Saviolakis GA, Melendez V, et al. Pharmacokinetic profiles of artesunate following multiple intravenous doses of 2, 4, and 8 mg/kg in healthy volunteers: phase 1b study. Malar J. 2012;11:255.View ArticlePubMedPubMed CentralGoogle Scholar
- Chotivanich K, Udomsangpetch R, McGready R, Proux S, Newton P, Pukrittayakamee S, et al. Central role of the spleen in malaria parasite clearance. J Infect Dis. 2002;185:1538–41.View ArticlePubMedGoogle Scholar
- Zhao KC, Song ZY. Distribution and excretion of artesunate in rats. Proc Chin Acad Med Sci Peking Union Med Coll. 1989;4:186–8.PubMedGoogle Scholar
- Newton P, Suputtamongkol Y, Teja-Isavadharm P, Pukrittayakamee S, Navaratnam V, Bates I, White N. Antimalarial bioavailability and disposition of artesunate in acute falciparum malaria. Antimicrob Agents Chemother. 2000;44:972–7.View ArticlePubMedPubMed CentralGoogle Scholar
- Li Q, Xie LH, Si Y, Wong E, Upadhyay R, Yanez D, Weina PJ. Toxicokinetics and hydrolysis of artelinate and artesunate in malaria-infected rats. Int J Toxicol. 2005;24:241–50.View ArticlePubMedGoogle Scholar
- Li QG, Peggins JO, Fleckenstein LL, Masonic K, Heiffer MH, Brewer TG. The pharmacokinetics and bioavailability of dihydroartemisinin, arteether, artemether, artesunic acid and artelinic acid in rats. J Pharm Pharmacol. 1998;50:173–82.View ArticlePubMedGoogle Scholar
- Berman J. MMV annual report: development of an intravenous artemisinin treatment for severe malaria. Discover, develop, deliver, medicines for malaria venture. 2001; p. 29–30.Google Scholar
- Grace JM, Skanchy DJ, Aguilar AJ. Metabolism of artelinic acid to dihydroqinqhaosu by human liver cytochrome P4503A. Xenobiotica. 1999;29:703–17.View ArticlePubMedGoogle Scholar
- LaCrue AN, Scheel M, Kennedy K, Kumar N, Kyle DE. Effects of artesunate on parasite recrudescence and dormancy in the rodent malaria model Plasmodium vinckei. PLoS ONE. 2011;6:e26689.View ArticlePubMedPubMed CentralGoogle Scholar
- Codd A, Teuscher F, Kyle DE, Cheng Q, Gatton ML. Artemisinin-induced parasite dormancy: a plausible mechanism for treatment failure. Malar J. 2011;10:56.View ArticlePubMedPubMed CentralGoogle Scholar
- White NJ, Nosten F, Looareesuwan S, Watkins WM, Marsh K, Snow RW, et al. Averting a malaria disaster. Lancet. 1999;353:1965–7.View ArticlePubMedGoogle Scholar
- Davis TM, Phuong HL, Ilett KF, Hung NC, Batty KT, Phuong VD, et al. Pharmacokinetics and pharmacodynamics of intravenous artesunate in severe falciparum malaria. Antimicrob Agents Chemother. 2001;45:181–6.View ArticlePubMedPubMed CentralGoogle Scholar
- White NJ. The parasite clearance curve. Malar J. 2011;10:278.View ArticlePubMedPubMed CentralGoogle Scholar
- Saunders D, Khemawoot P, Vanachayangkul P, Siripokasupkul R, Bethell D, Tyner S, et al. Pharmacokinetics and pharmacodynamics of oral artesunate monotherapy in patients with uncomplicated Plasmodium falciparum malaria in western Cambodia. Antimicrob Agents Chemother. 2012;56:5484–93.View ArticlePubMedPubMed CentralGoogle Scholar
- Bakshi RP, Nenortas E, Tripathi AK, Sullivan DJ, Shapiro TA. Model system to define pharmacokinetic requirements for antimalarial drug efficacy. Sci Transl Med. 2013;5:205ra135.View ArticlePubMedGoogle Scholar
- Zaloumis SG, Tarning J, Krishna S, Price RN, White NJ, Davis TM, et al. Population pharmacokinetics of intravenous artesunate: a pooled analysis of individual data from patients with severe malaria. CPT Pharmacometrics Syst Pharmacol. 2014;3:e145.View ArticlePubMedPubMed CentralGoogle Scholar
- Hawkes MT, Forgie S, Brophy J, Crockett M. Artesunate treatment of severe pediatric malaria: a review of parasite clearance kinetics and clinical implications. Can J Infect Dis Med Microbiol. 2015;26:237–40.PubMedPubMed CentralGoogle Scholar
- Centers for Disease Control. Guidelines for treatment of malaria in the United States. Atlanda: Centers for Disease Control and Prevention; 2013.Google Scholar