Inorganic nanoparticles kill Toxoplasma gondii via changes in redox status and mitochondrial membrane potential
Received 12 September 2016
Accepted for publication 22 November 2016
Published 28 February 2017 Volume 2017:12 Pages 1647—1661
Checked for plagiarism Yes
Review by Single anonymous peer review
Peer reviewer comments 3
Editor who approved publication: Dr Thomas J Webster
Oluyomi Stephen Adeyemi,1,2 Yuho Murata,1 Tatsuki Sugi,1 Kentaro Kato1
1National Research Center for Protozoan Diseases, Obihiro University of Agriculture and Veterinary Medicine, Obihiro, Japan; 2Medicinal Biochemistry and Toxicology Laboratory, Department of Biological Sciences, Landmark University, Omu-Aran, Nigeria
Abstract: This study evaluated the anti-Toxoplasma gondii potential of gold, silver, and platinum nanoparticles (NPs). Inorganic NPs (0.01–1,000 µg/mL) were screened for antiparasitic activity. The NPs caused >90% inhibition of T. gondii growth with EC50 values of ≤7, ≤1, and ≤100 µg/mL for gold, silver, and platinum NPs, respectively. The NPs showed no host cell cytotoxicity at the effective anti-T. gondii concentrations; the estimated selectivity index revealed a ≥20-fold activity toward the parasite versus the host cell. The anti-T. gondii activity of the NPs, which may be linked to redox signaling, affected the parasite mitochondrial membrane potential and parasite invasion, replication, recovery, and infectivity potential. Our results demonstrated the antiparasitic potential of NPs. The findings support the further exploration of NPs as a possible source of alternative and effective anti-T. gondii agents.
Keywords: antiparasite, drug screening, nanomedicine, toxoplasmosis
Toxoplasma gondii is an intracellular parasite belonging to the Apicomplexa family.1 T. gondii is the causative agent of toxoplasmosis, which is one of the most common parasitic diseases.2 Toxoplasmosis is common because the parasite has low host specificity and therefore can infect a range of hosts, including nearly one-third of the human population.3 Toxoplasma infection can be asymptomatic in healthy individuals but fatal in pregnant or immunocompromised individuals; it has been linked to abortion, fetal abnormalities, and encephalitis in these individuals.4 In healthy individuals who are infected with Toxoplasma, the multiplication of the parasites is handled by the immune system and the administered drugs, but cysts remain in all infected tissues, including the brain, thereby serving as a source for exacerbations. Therefore, efficient treatment of all infected cells to prevent cyst formation is imperative.
Current treatment options for toxoplasmosis patients are limited. They include the use of antimalarial drugs or antibiotics, which often cause significant side effects, including bone marrow suppression and rashes.4 Current therapy for toxoplasmosis suppresses the active infection but does not cure the latent infection and is poorly tolerated. Without prolonged suppressive treatment, up to 80% of cases relapse, and 20%–30% of patients on suppressive therapy relapse. The side effects of drugs have led to discontinuation of therapy in up to 40% of patients.3,5 Consequently, toxoplasmosis represents a large global burden that is further enhanced by the shortcomings of the current therapeutic options. These factors underscore the urgent need for better anti-Toxoplasma drugs and/or new approaches in the treatment of toxoplasmosis. An ideal anti-Toxoplasma drug would be potent, nontoxic, and able to eliminate latent infection.
There is expanding interest in deploying nanotechnology for biomedical purposes,6 and some reports suggest that nanoparticles (NPs) could form the bulk of future treatment strategies for various diseases.7,8 NPs are already being exploited for biomedical applications, due to their nanoscale size and other remarkable properties, including surface reactivity.9 These particles can produce reactive oxygen species (ROS) that have the ability to kill infectious agents.10,11 Furthermore, the small size of NPs allows them to transverse membrane barriers, leading to greater reactivity.12 In addition, NPs could be accumulated in tissues,13 thereby presenting a formidable platform to target T. gondii cysts in host tissues. Of special interest are the metal NPs such as gold and silver, which have antimicrobial activity,14,15 antiparasitic activity,16,17 and other bioactivities, including the selective inhibition of some enzyme activities.9,18–21 The versatility of metal NPs10 makes them an attractive choice to be explored further as antiparasitic agents, particularly against toxoplasmosis. Here, we explored the potential of metal NPs as novel anti-T. gondii agents using in vitro experimental infection models.
Materials and methods
Inorganic NPs, including gold NPs (AuNPs; 5 nm), silver NPs (AgNPs; 10 nm), and platinum NPs (PtNPs; 3 nm), were purchased from (Sigma-Aldrich, St Louis, MO, USA). The NPs were used as supplied following characterization to confirm the supplier’s specification. The NPs were reconstituted in fresh culture medium prior to each use. All reagents were of analytical grade and used as supplied unless otherwise stated.
In vitro anti-T. gondii potential of metal NPs
The T. gondii RH strain 2F22 was used for this study unless otherwise stated. The parasite was maintained by repeated passages in monolayers of human foreskin fibroblast (HFF) cells (American Type Culture Collection, Manassas, VA USA) cultured in Dulbecco’s Modified Eagle’s medium (DMEM; Nissui, Tokyo, Japan) supplemented with GlutaMAX™-I (Thermo Fisher Scientific Inc, St Louis, MO, USA), 10% (v/v) fetal calf serum (FCS; Gibco), and penicillin and streptomycin (100 U/mL; Thermo Fisher Scientific Inc). Host cells infected with T. gondii tachyzoites were passed through a 27 G needle to lyse them. The cell lysates were then filtered through a 5 μm filter to obtain a tachyzoite suspension free of host cell debris. The suspension was washed with fresh culture medium. Then, the parasite density was measured using a hemocytometer and adjusted for in vitro experimental infection analysis.
In vitro invasion and growth inhibition assessment by luciferase reporter assays
The number of T. gondii tachyzoites was determined using a luminescence-based assay of β-galactosidase (β-gal) activity expressed by the parasite strain RH-2F. To obtain a purified parasite suspension for the assays, infected cells were syringe released and the lysates were filtered to remove cell debris.
First, the anti-T. gondii EC50 and IC50 values for host cell toxicity were determined. In this preliminary assay, the NPs (AuNPs, AgNPs, and PtNPs) were screened at various concentrations ranging from 0.01 to 1,000 μg/mL. Based on the preliminary results, further experimental screening was done using concentrations of 15, 10, and 1,000 μg/mL for AuNPs, AgNPs, and PtNPs, respectively.
The growth inhibition assays and in vitro invasion assays were performed as described by Ishiwa et al.22 For the growth inhibition assay, purified parasite suspension was added to growing monolayers and invasion was allowed to occur for 1 h. The medium was then removed, the monolayers were washed thoroughly, and fresh medium containing the NP solutions (reconstituted in culture medium) was added. The monolayers were then incubated for 48 h. For the invasion assay, purified parasite suspension and the NP solutions (AuNPs, AgNPs, and PtNPs freshly reconstituted in culture medium) were added to the growing monolayers and incubated for 1 h to allow for invasion. The medium was then removed, the monolayers were washed thoroughly to remove uninvading parasites, and fresh medium was added. The monolayers were then incubated for 48 h. To assay invasion and growth inhibition, purified parasite suspension and the NP solutions (reconstituted in culture medium) were added to the growing monolayers and incubated for 48 h. The mock-treated (treatment with NP vehicle; in this case, culture medium) cells served as a positive control, whereas the medium-only well was used to correct for any background signal noise. After 48 h incubation at 37°C in a 5% CO2 atmosphere, the viability of the RH-2F parasite strain was determined by assaying for galactosidase expression using a Beta-Glo® Luminescent Assay kit (Promega, Madison, WI, USA). The assay was performed in triplicate and repeated three times. All experiments were performed in 96-well optical bottom plates (Nunc; Fisher Scientific, Pittsburgh, PA, USA) unless otherwise stated.
Host cell viability
Cytotoxicity of metal NPs in mammalian cells
HFF cells were maintained in DMEM supplemented with GlutaMAX™-I, 10% (v/v) FCS, and penicillin and streptomycin (100 U/mL). Cells were grown to confluence at 37°C in a 5% CO2 atmosphere. All experiments were performed in 96-well plates (Nunc) unless otherwise stated. At confluence, cells were trypsinized and resuspended to the desired cell density. The cells were seeded onto plates at a density of 1×105 cells/well and incubated for 72 h followed by treatment with various concentrations (between 0.01 and 1,000 μg/mL) of the NPs (AuNPs, AgNPs, and PtNPs). Culture medium lacking the test compounds was added to the control well, and the medium only well was used to correct for any background signal noise. The treated cells were incubated for 72 h before being subjected to the cell viability assay. All experiments were performed in 96-well plates (Nunc) unless otherwise stated.
Cell viability was determined using the CellTiter 96® AQueous One Solution Cell Proliferation Assay kit (Promega). Briefly, the well plate and its contents were equilibrated to room temperature. Then, 20 μL of the CellTiter 96® AQueous One reagent was added to each well. The contents were briefly mixed on an orbital shaker and then incubated at 37°C in a 5% CO2 atmosphere for 1–4 h. The absorbance signal was recorded at 490 nm using a microplate reader (MTP-500; Corona Electric, Hitachinaka, Japan). The assay was repeated three times in triplicate. The results are given as the mean ± standard error of the mean (SEM; n=3) of three independent experiments.
Invasion and intracellular replication assessment by immunofluorescence (IF) staining
Invasion assays were performed as described by Kieschnick et al23 and Sugi et al.24 Briefly, freshly harvested and purified parasites (1×105) were inoculated onto a monolayer of HFF cells on a coverslip for 1 h at 37°C with the different NP solutions (reconstituted in fresh medium prior to use) or medium only to serve as mock treatment. Following invasion, the cells were washed three times with ice-cold PBS, and extracellular parasites were stained with rabbit anti-T. gondii RH strain polyclonal antibodies (1:1,000) (Bio-Rad Laboratories, Hercules, CA, USA) in PBS containing 2% FCS for 30 min on ice. The cells were then washed three times with PBS containing 2% FCS, fixed with 4% paraformaldehyde in PBS, and permeabilized with ice-cold methanol for 20 min. Then, the cells were washed three times with 2% FCS–PBS and further stained with monoclonal mouse anti-SAG1 antibodies (1:1,000) (HyTest, Turku, Finland) in PBS containing 2% FCS. Secondary staining was achieved by antibody solutions containing Alexa 488 goat antimouse and Alexa 594 goat antirabbit and DAPI for nuclear staining (1:1,000) in 2% FCS–PBS. The cells were visualized with a fluorescence microscopy (Eclipse E400; Nikon, Tokyo, Japan). At least 50 microscopic fields were chosen at random; extracellular parasites were detected using the rabbit anti-Toxoplasma antibodies, and the total parasites were detected with the mouse anti-SAG1 antibodies.
Intracellular replication assessment by IF staining
Intracellular replication assays were performed as described by Sugi et al.24 Briefly, purified parasites (1×105) were inoculated onto growing HFF monolayers on a coverslip and incubated at 37°C for 1 h to allow invasion. Cells were washed three times with warm culture medium to remove uninvaded parasites and were then incubated for different time periods (12, 16, 18, and 24 h) in medium containing NP solutions or medium only (mock treatment). After each incubation time period, the cells were fixed with 4% paraformaldehyde in PBS for 30 min at room temperature, permeabilized with ice-cold methanol for 20 min at room temperature, and then washed three times with PBS. The cells were blocked with 2% BSA in 0.1% Tween 20–PBS for 1 h at room temperature. The primary antibody, monoclonal mouse anti-SAG1 (1:1,000) in blocking buffer (0.1% Tween 20–PBS), was added and incubated for 30 min at 37°C. The cells were then washed three times (5 min between each wash) with blocking buffer. Secondary antibody solutions containing Alexa 546 goat antimouse and DAPI for nuclear staining in blocking buffer were added and incubated for 30 min at 37°C. Coverslips were washed three times with PBS and viewed by fluorescence microscopy (Eclipse E400). At least 50 microscopic fields were chosen at random to count the parasitophorous vacuoles. Average numbers of tachyzoites per vacuole were calculated.
The reversibility of effect was assessed as described by Kamau et al.4 Briefly, invading parasites were grown in the presence of NP solutions (reconstituted in culture medium) for 12 and 24 h. The medium was removed, and the monolayer was washed thoroughly before adding fresh medium. The plate was then incubated in the absence of the NPs for another 24 h, and the growth curve was determined by measuring the β-gal activity using the luminescent reporter assay. In parallel, after each incubation (12 and 24 h) of invading parasites in the presence of the NP solutions, parasite viability was determined on the basis of luminescence to compare and evaluate the ability of the parasites to recover from the treatment. Three independent assays were performed.
Infectivity and likely cellular target
A procedure previously described by Kamau et al4 was used. In brief, freshly lysed and purified parasites were treated for either 24 or 48 h at 37°C in 5% CO2 with either medium only or an NP solution (reconstituted in culture medium) and then washed three times with culture medium to remove the NPs. The treated parasites were used to infect fresh HFF monolayers by incubating them with the cells for 48 h, prior to assaying for growth using the luminescence reporter assay. Extracellular parasites were incubated with the various NPs for 12 h after which the parasites were harvested and used for infectivity tests as described earlier.
To determine whether effects on parasite growth were due to effects on the host cell, uninfected HFF monolayers were pretreated for 24 h at 37°C in 5% CO2 with either medium only or an NP solution. The pretreated host monolayers were washed thoroughly with fresh medium. Freshly lysed and purified parasites were then allowed to invade the pretreated monolayers for 4 h, the monolayer was washed three times with medium, and parasite growth was allowed to proceed for 24 h. Growth curves were determined using the luminescence reporter assay. In parallel, media-pretreated host cell monolayers were infected with parasites in a similar fashion, but the NP solutions were added 4 h postinvasion and incubated for 24 h. This allowed comparisons of the effects of the NPs after pretreatment to the effects of having the NPs present for the entire incubation period.
Measurement of intracellular ROS
Measurement of intracellular ROS was based on the intracellular peroxide-dependent oxidation of 2′,7′-dichlorodihydrofluorescein diacetate (H2DCF-DA; Sigma, St Louis, MO, USA) to form the fluorescent compound 2′,7′-dichlorofluorescein (DCF), as previously described by Warleta et al.25 Briefly, growing HFF monolayers were infected with purified parasite suspension and incubated for 24 h at 37°C. Subsequently, the parasite-infested HFF cells were treated with the NPs and further incubated for 8 h at 37°C. The parasites were then harvested, purified, and resuspended in PBS containing the H2DCF-DA to a final concentration of 100 μM. The parasite suspension containing the fluorescent dye was incubated for 30–60 min at 37°C. Fluorescence acquisition was then assessed using a spectrofluorometer (Corona Electric) with excitation set at 485 nm and emission at 530 nm. H2O2 was included as a positive control.
Measurement of the mitochondrial membrane potential
The measurement of mitochondrial membrane potential was acquired by spectrofluorimetry according to a procedure described by Baracca et al.26 Briefly, growing HFF monolayers were infected with purified parasite suspension and incubated for 24 h at 37°C. The parasite-infested HFF monolayers were treated with the NPs and further incubated for 8 h at 37°C. The parasites were then harvested, purified, and stained with 200 nM MitoRed (Dojindo Molecular Technologies Inc, Kumamoto, Japan) by following the manufacturer’s protocol. Fluorescence acquisition was assessed using a spectrofluorometer with excitation set at 560 nm and emission at 580 nm.
Data were analyzed using a one-way ANOVA (GraphPad Software Inc, San Diego, CA, USA) and are presented as the mean ± SEM. Comparisons among groups were determined using a one-way ANOVA and Dunnett’s posttest. P-value <0.05 was considered to be statistically significant. The EC50 was estimated by plotting NP concentrations versus the percentages of T. gondii viability, and the IC50 was estimated by plotting NP concentrations versus the percentages of cell viability. All the experiments were developed in the same conditions thrice separately, and the results were expressed as the mean ± SEM. Selectivity indexes (SIs) were also estimated. The analyses were carried out using Prism 5 (Graphpad Software Inc), whereas nonlinear regression analysis was used to fit the curve. All experiments were performed in triplicate and carried out three times independently unless otherwise stated.
NPs significantly reduced the parasite growth
In our preliminary experiments, we sought to establish the antiparasitic activity and host cell cytotoxic potential of the metal NPs. Therefore, first, we screened the NPs (AuNPs, AgNPs, and PtNPs) at various concentrations between 0.01 and 1,000 μg/mL for anti-T. gondii activity by incubating freshly lysed and purified parasites with the NPs in growing monolayers for 48 h. Parasite growth curves were determined by measuring the β-gal activity of the viable parasites using a luciferase reporter assay. The NPs significantly reduced the parasite viability by >90% (Figure 1) with EC50 values of ≤7, ≤1, and ≤100 μg/mL for AuNPs, AgNPs, and PtNPs, respectively (Table 1). AuNPs and AgNPs showed a stronger anti-T. gondii activity relative to that of PtNPs, consistent with other studies,14–17 that have reported antimicrobial and/or antiparasitic properties of AuNPs and AgNPs; similar studies using PtNPs were scarce in the literature. A reference drug (sulfadiazine, used to treat active toxoplasmosis), which was included as a positive control, decreased the parasite viability by >95%. This is consistent with published data27 and thus supports the validity of our screening assay. The estimated IC50 values in our host cell cytotoxicity studies were ≥260, ≥48, and ≥2,000 μg/mL for AuNPs, AgNPs, and PtNPs, respectively. Estimation of the ratio of the host cell cytotoxic IC50 value to the antiparasite EC50 value as a measure of the therapeutic or SI was promising, with the SIs of ≥30, ≥40, and ≥20 for AuNPs, AgNPs, and PtNPs, respectively. Having established the EC50 values for the NPs, we performed further experiments using the single concentrations of 15, 10, and 1,000 μg/mL for AuNPs, AgNPs, and PtNPs, respectively, unless otherwise stated. Having determined that the NPs at these concentrations showed no host cell toxicity (Figure 2A), we screened them at these concentrations for T. gondii growth inhibition using the β-gal expressing luciferase reporter system. The results showed that the NPs induced >90% growth inhibition (Figure 2B). Next, we sought to determine whether the parasite invasion and growth processes were affected by treatment with NPs, using the luciferase reporter assay system. The data revealed that the NPs reduced parasite growth by >60% (Figure 2C) and suggest that the NPs may act during the parasite invasion window. This finding could serve as an indirect measure of the parasite invasion efficiency in the presence of NPs. The data from the invasion and growth assay, in which the NPs were present throughout the 48 h incubation period, showed a >90% reduction in parasite viability relative to mock treatment (Figure 2D). The results are similar to those obtained for the growth only assay, in which the purified parasites were allowed to invade the host monolayers for 1 h before the addition of the NPs. To further confirm that the NPs have a direct anti-T. gondii activity, we incubated freshly lysed and purified parasites with the NPs for 12 h extracellularly. Relative to the mock treatment, the NPs significantly (P<0.05) reduced the parasite viability (Figure 2E), comparable to the results obtained when the parasite viability screening was done using the host monolayer, lending credence to the antiparasitic action of the NPs. Efforts to determine whether the NPs were inducing cyst formation rather than killing the parasite (using CST1 staining; data not shown) revealed the absence of cyst formation and thus supported the concept that treatment with NPs killed the parasites.
Poor infectivity and recovery following NP treatment
First, we sought to assess whether the NP-treated parasites could sustain their ability to infect fresh host monolayers. Freshly lysed and purified parasites were incubated with the NPs in growing host monolayers for 24 and 48 h. At each time point, the parasites were harvested and used to infect fresh host cells. After 48 h incubation, the parasite viability was determined. The results showed that treatment with the NPs at both time points negatively (P<0.05) impacted parasite infectivity (Figure 3A and B). NP treatment produced a >75% reduction in parasite infectivity potential relative to mock treatment. In parallel, for comparison, we determined the parasite infectivity potential using extracellular parasites exposed to the NPs for 12 h. The data showed a similar trend of significant depression of the parasite infectivity by the NPs (Figure 3C). This finding thus confirms the antiparasitic action of the NPs. The poor infectivity potential exhibited by the parasites after treatment with the NPs could indicate unlikely reversible antiparasitic actions. Therefore, we evaluated whether the antiparasitic effect of NPs was reversible. Freshly lysed and purified parasites were incubated with the NPs in growing host monolayers for 12 and 24 h. At each time point, the NPs were removed and replaced with fresh medium, and the plates were incubated for a further 24 h after which parasite viability was determined. In parallel, parasite viability at 12 and 24 h of NP or mock treatment was determined to serve as the baseline for comparison. The data revealed a marginal recovery of <10% following 24 h of NP treatment. Conversely, a slightly higher recovery of <25% was observed for the 12 h NP treatment (Figure 4A and B). These data suggest that the NPs exhibit a minimally reversible but time-dependent antiparasitic action. It thus appears that the incubation time of the NPs with the parasites may play a role in determining whether the antiparasitic action may be reversible. Overall, our results indicate that the poor parasite infectivity potential may preclude the reversibility of the antiparasitic effects of the NPs.
The antiparasitic action of the NPs may be due, in part, to a parasite target
We then sought to determine whether the NPs affected parasite viability through a host or parasite target. Growing host cell monolayers were pretreated with the NPs for 24 h, and then freshly lysed and purified parasites were allowed to infect the pretreated host cells. After 24 h incubation, the parasite viability was determined. The data revealed >75% parasite growth in the host cells pretreated with the NPs relative to the mock pretreatment (Figure 4C). Although these findings suggest that the antiparasitic effects of NPs may be linked to a parasite target, we could not rule out the possibility that a host cell target also contributed to the observed anti-T. gondii activity of NPs. Of note, T. gondii growth in the host monolayers pretreated with AuNPs and PtNPs was significantly reduced by ≤20%.
NPs affect parasite invasion and replication
Toward unraveling the mode of the antiparasitic action of NPs, we sought to determine whether any stage of the parasite lytic cycle was affected by the NPs. The parasite lytic cycle involves the following three repeated stages: invasion, replication, and egress. We assessed the effect of NPs on invasion and intracellular replication. The IF staining was used to assess the ability of the parasites to invade growing host monolayers and to determine the parasite number per vacuole in the presence of the NPs. The results revealed a significant reduction in parasite ability to invade growing host monolayers by >65, >60, and >50% for AuNPs, AgNPs, and PtNPs, respectively (Figure 5A). Similarly, the NPs caused >67% depletion in the average replication of parasites per vacuole (at least 100 vacuoles were counted per experiment) relative to the mock treatment (Figure 5B). These findings corroborate the data obtained from the invasion and growth assays using the luciferase reporter systems in which the NPs caused a >90% parasite growth inhibition. Further analyses at different time points (12, 16, 18, and 24 h) showed that NP treatment resulted in a time-dependent reduction in the number of parasites per vacuole (Figure 6A–D). Moreover, the highest number of parasites per vacuole was <8 for the NPs relative to the mock treatment, for which the parasite number steadily increased with incubation time.
In support of the time-dependent depression of the capacity of the parasites to replicate, at the 24 h time point, the treatment with the NPs led to <4 parasites per vacuole (Figure 7A–C), which was in stark contrast to the mock treatment, where the number of parasites per vacuole gradually advanced to >24.
Anti-T. gondii activity of NPs may be linked to altered redox status via intracellular production of ROS
Having established that the NPs possess anti-T. gondii activity, we sought to understand their likely mode of the antiparasitic action. First, we tested whether ROS play a role in the parasite killing capability of the NPs. In this experiment, we added an antioxidant, Trolox, to the NP antiparasite screening assay. The data showed that the antiparasitic effect of the NPs was mitigated in the presence of Trolox (Figure 8A–C). Although at the highest concentration (1,000 μg/mL), the addition of Trolox had no visible effect on the antiparasitic action of PtNPs. Nonetheless, the results indicate that the EC50 values for the NPs were increased in the presence of Trolox compared to that in the absence of Trolox. These findings implicate oxidative stress in the anti-T. gondii effect of the NPs. Although the reversal of the antiparasitic action of NPs through the addition of Trolox indicated a connection to oxidative stress, it was not a direct evaluation of the production of ROS. Therefore, we sought to directly determine whether ROS was produced during NP treatment of T. gondii. We monitored the production of ROS using H2DCF-DA, a cell-permeable reduced fluorescein that is nonfluorescent until its acetate groups are removed by intracellular esterases during oxidation. Our results showed that AgNPs and PtNPs caused >100% ROS production relative to the nontreated control (Figure 9A and B). Similar results (>200% over the untreated control) were obtained following H2O2 treatment (data not shown), validating the ROS detection assay. Conversely, the level of ROS production induced by AuNP treatment was higher than the untreated control but not statistically significant. We then asked whether the NP-induced ROS production was sustained after removing the NPs. The results showed that ROS production was sustained following treatment with AuNPs or AgNPs for 12 h after removing the NPs, suggesting that these NPs had a negative impact on the parasites.
NPs decrease the parasite mitochondrial membrane potential
The mitochondria represent a major source of ROS in the cell. Indeed, mitochondria are considered as the major target of excess cellular ROS. We therefore asked whether NP-induced ROS production affected the parasite mitochondria. We used MitoRed to evaluate the parasite mitochondrial membrane potential. MitoRed is a rhodamine-based dye that permeates cell membranes. It localizes in mitochondria and emits fluorescence. The interaction of MitoRed with the mitochondria is dependent on the membrane potential of the mitochondria. The 8 h treatment with the NPs led to reduced fluorescence intensity (Figure 10A and B), suggesting low accumulation of the rhodamine-based dye in the parasite mitochondria. This finding may indicate that the treatment with the NPs affected the parasite mitochondria by decreasing their membrane potential. It was also found that 12 h after the NPs had been removed, the parasites may not have recovered from the NP-induced reduction in their mitochondrial membrane potential. This finding further supports the antiparasitic impact of NP treatment on parasite mitochondria.
Our study demonstrates that AuNPs, AgNPs, and PtNPs have a promising anti-T. gondii activity without detectable host cell toxicity. We obtained antiparasite EC50 values of <7, <1, and <100 μg/mL for AuNPs, AgNPs, and PtNPs, respectively. Although the published reports of the antimicrobial and/or antiparasitic properties of PtNPs are limited, the EC50 values obtained in our study are well within the range of those reported elsewhere16,17,28–30 for the antimicrobial and/or antiparasitic action exhibited by AuNPs and AgNPs. Interestingly, a few of the studies17,29,30 reporting the antiparasitic activities of NPs revealed that under the same conditions, AgNPs had a lower EC50 value relative to that of AuNPs. A similar trend was observed in our studies that supports and further strengthens the promising antiparasitic potential of AuNPs and AgNPs. However, for PtNPs, a higher concentration was required to demonstrate the commensurate effective anti-T. gondii activity. The absence of appreciable host cell toxicity induced by the NPs at the effective anti-T. gondii concentrations supports further exploration of the selective antiparasitic action of NPs. The estimated therapeutic or SI revealed ≥13-fold more activity against the parasite versus the host cell for AuNPs and AgNPs, whereas it was ≥7 for PtNPs. This fact coupled with the absence of host cell toxicity induced by the NPs at the effective anti-T. gondii concentrations as well as the ≥75% parasite growth in host monolayers pretreated with the NPs suggests that these NPs have a partially selective antiparasitic action. Moreover, findings obtained when extracellular tachyzoites were incubated for 12 h with the NPs not only reinforce that the NPs have anti-T. gondii activity but also confirm previous reports16,17 demonstrating the antiparasitic potential of NPs. In addition, the poor recovery of parasites as well as the marginal parasite infectivity after treatment with NPs supports the further exploration of NPs as anti-infective agents. Together, these data show that NPs have favorable anti-T. gondii potential and thus support several earlier reports that demonstrated the anti-Cryptosporidium parvum,28 antileishmanial,16 antifilarial,30 antitrypanosomal, and antimalarial activities17 of AgNPs as well as the antiparasitic activity of AuNPs.17,30 However, this is the first report to show that AuNPs, AgNPs, and PtNPs can cause the death of T. gondii both within the host cell and extracellularly. Our findings attest to the promising potency of the NPs as antimicrobial,14,15 antiparasitic,17,29,30 and bioactive agents,8,9,18,31 and may herald a turning point or revolution in pharmacological therapy for parasitic infections.
Our data confirm that NPs significantly impact the invasion and replication stages of the parasite lytic cycle. These findings are preliminary and may represent early insights into how NPs restrict parasite growth. Although we do not yet know how or which of the processes that lead to parasite invasion of the host cell were impeded by the NPs (eg, association with the host plasma membrane, attachment to the host membrane, and host cell penetration32), our data provide evidence of a time-dependent reduction in parasite vacuoles and in the number of parasites per vacuole, which, if considered together, suggest that treatment with NPs arrests T. gondii replication rather than slowing it. We are of the opinion that the depleting numbers of parasite vacuoles were unlikely to be a result of premature egress by parasites from the host cell because the host cell numbers did not appear to diminish and extracellular parasites were not observed. These findings suggest that the NPs may have induced a host cell-mediated clearance of intracellular parasites through as yet unknown mechanisms.
Our findings also showed a significant reduction in the capacity of the parasites to successfully infect a fresh host after 24 or 48 h treatment with NPs, even though our data suggest that the antiparasitic effects of NPs may be marginally reversible. The NP-induced paralysis of the potential of parasites to successfully infect fresh host monolayers is not unexpected because it is compatible with previously documented findings of the anti-infective potential of NPs.10,11 It is possible that the poor parasite recovery following NP treatment stems from an NP-induced impact on parasite capacity for successful invasion and to a larger extent parasite infectivity. Our data imply that the anti-T. gondii action of NPs may be partially linked to their ability to affect the invasion and replication stages of the parasite lytic cycle. Taken together, the antiparasitic actions displayed by the NPs in this study are consistent with published findings on the antimicrobial actions of the NPs reviewed by Yah and Simate33 and support the concept of exploring NPs as promising alternative anti-T. gondii agents.
Because nanomedicine is still in its infancy, the antimicrobial and/or antiparasitic mode of action of the NPs is largely unknown. Our findings presented here implicate intracellular ROS in the parasite killing action of the NPs. The reversal of the antiparasitic action of NPs by Trolox suggested the involvement of oxidative stress in NP-induced killing of T. gondii; however, ROS measurement through the use of a fluorescent probe provided direct evidence that NP treatment promoted ROS production with a consequent contribution to NP-induced parasite death. These findings are consistent with the few reports that have shown that ROS generation by NPs, including AgNPs and AuNPs, is damaging, leading to the death of Leishmania major29 and causing the apoptotic killing of Filaria parasites.30
The lack of significant ROS production by AuNPs relative to the control may indicate that AuNP-induced ROS production was not a sudden burst of ROS production but rather a more extended process than that induced by AgNP or PtNP treatment. This concept is supported by the fact that after the NPs had been removed for 12 h, ROS production due to AuNP treatment steadily increased. This finding demonstrates a connection between oxidative affront and the parasite killing potential of AuNPs. Furthermore, the finding that the ROS production induced by AuNPs and AgNPs was sustained for 12 h after removing the NPs indicates that the oxidative stress caused by the NP treatment may have resulted from extended generation of ROS rather than an immediate burst of ROS. The sustained oxidative stress may have been responsible for the growth arrest as well as for the death of the parasite. The sustained oxidative onslaught would be very injurious, causing appreciable damage to cellular biomolecules, and may fuel the antiparasitic potency of the NPs. In contrast, the ROS production after the removal of PtNPs for 12 h showed a drastic decline. At the moment, we may not be able to explain the reason for this observation. Nonetheless, the protection afforded by the addition of Trolox strongly accentuated the role of oxidative insult in the antiparasitic action of the NPs. Furthermore, the NP-induced ROS production after the removal of the NPs adds evidence in support of the antiparasitic effects of these NPs. Taken together, our findings indicate that the antiparasitic action of the NPs could, in part, be linked to the altered redox status possibly via ROS production. This would not be unexpected given existing reports demonstrating the in vitro and in vivo ROS-generating potential of inorganic NPs, including AuNPs and AgNPs.12,29,30 Our data are in full accord with the ROS-inducing anti-infective character of NPs.10,11
In addition, our finding that treatment with NPs depleted the parasite mitochondrial membrane potential further reinforces our evidence for intracellular ROS production and its culpability in the antiparasitic action. The NP-induced decrease in the parasite mitochondrial membrane potential was sustained, even up to 12 h after the NPs had been removed. These data are consistent with the recent findings of Charvat and Arrizabalaga,34 which indicated that oxidative stress as a consequence of excess cellular ROS production was devastating to the parasite mitochondrial membrane potential and led to the death of T. gondii. Furthermore, these findings are consistent with several other reports that have shown that mitochondria are negatively affected by excess cellular ROS production, whereby ROS induces cell death by either promoting intrinsic apoptotic processes and/or activating cellular autophagy,35–37 all of which are possible routes to cell death as a result of NP-induced ROS production and/or altered redox status.
The finding that T. gondii succumbed to an NP-induced oxidative onslaught provides further evidence to strengthen the support for exploring compounds that can induce oxidative affront and/or interfere with parasite redox biology as a viable approach for the development of antiparasitic agents.
Our findings identify AuNPs, AgNPs, and PtNPs as promising anti-T. gondii candidates. To our knowledge, this is the first evidence of anti-T. gondii activity by AuNPs, AgNPs, and PtNPs. Furthermore, the antiparasitic action of these NPs could be linked, in part, to altered redox status via ROS production. These novel findings add to the growing body of data supporting the need to explore the potential of NPs within the nanomedical community. Further investigations, including in vivo evaluation as well as assessments of the anti-T. gondii potential of surface-modified NPs, are ongoing with a view toward developing a new and effective treatment strategy for acute and/or latent toxoplasmosis.
The study was funded through a Japan Society for the Promotion of Science (JSPS) Fellowship to Dr OS Adeyemi. This study was supported by grants-in-aid for Young Scientists, Exploratory Research, and Scientific Research on Innovative Areas (3308 and 3407) from the Ministry of Education, Culture, Science, Sports, and Technology (MEXT) of Japan; by the Program to Disseminate Tenure Tracking System and the Adaptable & Seamless Technology Transfer Program through Target-driven R&D (A-STEP) from the Japan Science and Technology Agency (JST); by the Ito Foundation; and by the Promotion for Young Research Talent and Network from Northern Advancement Center for Science & Technology (NOASTEC). The authors appreciate Dr Daisuke Kondoh of the Obihiro University of Agriculture and Veterinary Medicine, Japan, for providing assistance with electron microscopy.
The authors report no conflicts of interest in this work.
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