- Open Access
Evaluation of in vitro antileishmanial efficacy of cyclosporin A and its non-immunosuppressive derivative, dihydrocyclosporin A
Parasites & Vectors volume 13, Article number: 94 (2020)
New therapeutic drugs are urgently needed against visceral leishmaniasis because current drugs, such as pentavalent antimonials and miltefosine, produce severe side effects and development of resistance. Whether cyclosporine A (CsA) and its derivatives can be used as therapeutic drugs for visceral leishmaniasis has been controversial for many years.
In this study, we evaluated the efficacy of CsA and its derivative, dihydrocyclosporin A (DHCsA-d), against promastigotes and intracellular amastigotes of Leishmania donovani. Sodium stibogluconate (SSG) was used as a positive control.
Our results showed that DHCsA-d was able to inhibit the proliferation of L. donovani promastigotes (IC50: 21.24 μM and 12.14 μM at 24 h and 48 h, respectively) and intracellular amastigotes (IC50: 5.23 μM and 4.84 μM at 24 and 48 h, respectively) in vitro, but CsA treatment increased the number of amastigotes in host cells. Both DHCsA-d and CsA caused several alterations in the morphology and ultrastructure of L. donovani, especially in the mitochondria. However, DHCsA-d showed high cytotoxicity towards cells of the mouse macrophage cell line RAW264.7, with CC50 values of 7.98 μM (24 h) and 6.65 μM (48 h). Moreover, DHCsA-d could increase IL-12, TNF-α and IFN-γ production and decrease the levels of IL-10, IL-4, NO and H2O2 in infected macrophages. On the contrary, CsA decreased IL-12, TNF-α, and IFN-γ production and increased the levels of IL-10, IL-4, NO and H2O2 in infected macrophages. The expression of L. donovani cyclophilin A (LdCyPA) in promastigotes and intracellular amastigotes and the expression of cyclophilin A (CyPA) in RAW 264.7 cells were found to be significantly downregulated in the CsA-treated group compared to those in the untreated group. However, no significant changes in LdCyPA and CyPA levels were found after DHCsA-d or SSG treatment.
Our findings initially resolved the dispute regarding the efficacy of CsA and DHCsA-d for visceral leishmaniasis treatment. CsA showed no significant inhibitory effect on intracellular amastigotes. DHCsA-d significantly inhibited promastigotes and intracellular amastigotes, but it was highly cytotoxic. Therefore, CsA and DHCsA-d are not recommended as antileishmanial drugs.
Visceral leishmaniasis (VL), a significantly neglected disease, is a systemic and chronic disease. Severe zoonosis occurs due to infections with Leishmania donovani or L. infantum. Worldwide, recurrent epidemics of VL have caused high morbidity and mortality in affected communities in 88 countries, with an estimated 400,000 new cases and 20,000 to 40,000 associated deaths . VL is even now prevalent in China, in the Gansu, Sichuan, Qinghai and Shanxi Provinces and the Xinjiang Uygur Autonomous Region . Pentavalent antimonials (SbV) have been used as a first choice of treatment for VL in China, but currently the development of resistance against antimonials has become serious, and the severe effects of sodium stibogluconate, another anti-leishmanial drug, on the heart, liver and pancreas cannot be ignored . Similar to antimonials, anti-Leishmanial drugs, such as amphotericin B, miltefosine and pentamidine, are also associated with severe side effects and resistance due to their long half-lives . Thus, new therapeutic drugs are urgently needed.
It has always been controversial whether the immunosuppressor cyclosporin A (CsA) and its non-immunosuppressive derivatives can be used to treat VL. CsA displays anti-microbial activity against a variety of protozoan pathogens, such as Toxoplasma and Trypanosoma brucei [5, 6]. CsA has also been employed to inhibit Leishmania species. Previous studies have suggested that CsA has damaging effects on Leishmania tropica [7, 8] and L. major  in vivo and extracellular promastigotes of L. tropica were found to be sensitive to CsA . Meanwhile, CsA was found to have a dose-dependent inhibitory effect on the growth of both L. donovani promastigotes and axenic amastigotes . In addition, CsA was found to have a desired effect on VL in clinical cases . It was considered to be highly efficacious in treating cytophagic histiocytic panniculitis and haemophagocytic lymphohistiocytosis, triggered by a previous visceral Leishmania infection, after failure of treatment with drugs, such as high-dose glucocorticoids, anakinra and etoposide . However, CsA treatment was observed to convert the L. donovani-infected “cure” C57BL/10 mouse phenotype to a “noncure” phenotype . Further, these mice exhibited a significant increase in the level of infection after 15 days of CsA-treatment , and the number of infected macrophages and amastigotes per macrophage in CsA-treated mice was significantly increased . Based on these controversial results, we thought that CsA might inhibit the viability and proliferation of Leishmania promastigotes and host-free amastigotes in vitro and that CsA would likely play a prominent role in leishmanial infection in animals. Therefore, we hypothesized that the effect of CsA inhibition on intracellular amastigotes of L. donovani is counteracted by its immunosuppressive effect.
CsA exhibits its immunosuppressive action by inhibiting the production of calcineurin through binding to its intracellular specific receptor, cyclophilin A (CyPA) [16, 17]. Leishmania donovani can also express a variant of CyPA, known as L. donovani cyclophilin A (LdCyPA) [18, 19], whose structural and biological functions are different from those of human CyPA. LdCyPA was shown to play a pivotal role in the survival and persistence of parasites in infected tissues . Thus, the inhibitory efficacy of CsA towards intracellular amastigotes can be indirectly verified by changes in the expression levels of CyPA and LdCyPA.
Dihydrocyclosporin A (DHCsA-d), which is a closely related co-metabolite of CsA , has been reported to exert only marginal immunosuppressive activity and has been used as a control to determine the role of immunosuppression in the pharmacology of CsA-based treatment of parasitic infections . Interestingly, DHCsA-d was found to also inhibit parasites in vivo and in vitro . Therefore, we aimed to explore whether DHCsA-d could be used as an inhibitor of L. donovani.
In this study, promastigotes and intracellular amastigotes were subjected to treatment with CsA, DHCsA-d, or sodium stibogluconate (SSG) to find their effective 50% inhibitory concentrations. Next, changes in the morphology and ultrastructure of L. donovani promastigotes and intracellular amastigotes were assessed and cytokine and nitric oxide (NO)/hydrogen peroxide (H2O2) production by the cells was detected after CsA, DHCsA-d, or SSG treatment. Finally, the expression of LdCyPA in promastigotes and intracellular amastigotes and the expression of CyPA in RAW 264.7 cells that were cultured in the presence of CsA, DHCsA-d, or SSG were detected using western blotting to verify the efficacy of DHCsA-d and CsA against L. donovani promastigotes, intracellular amastigotes and cells.
Leishmania donovani strain MHOM/CN/IN/80/DD8 was used in this study . Leishmania promastigotes in the logarithmic phase were cultured at 28 °C in M199 medium at pH 7.4 (Sigma-Aldrich, Saint Louis, MO, USA), supplemented with 10% fetal bovine serum (Hyclone, Logan, UT, USA) and antibiotics (Pen-Strep, 100 U/ml penicillin-100 μM streptomycin sulphate).
Stibogluconate sodium (MCE, Monmouth Junction, NJ, USA) was dissolved in saline to prepare a 20 mM stock. Cyclosporin A (ApexBio, Houston, TX, USA) and dihydrocyclosporin A (TRC, North York, ON, CA) were dissolved in a 20 mM stock of dimethyl sulfoxide (DMSO) (Sigma-Aldrich). For experiments, the DMSO concentration in the culture medium did not exceed 0.1%.
In vitro inhibitory assays
Promastigotes, in logarithmic phase, were grown at a cell density of 1.0 × 106 cells/ml, CsA, DHCsA-d, or SSG was added at different concentrations prepared from concentrated stock solutions: 5, 10, 15, 20 and 25 μM for CsA ; 5, 10, 15, 20 and 25 μM for DHCsA-d ; and 5, 10, 25, 50 and 90 μM for SSG . Parasite inhibition rates were evaluated at 24 h and 48 h using flow cytometry, employing an FITC Annexin V Apoptosis Detection Kit I (BD, Franklin Lakes, NJ, USA), according to the manufacturer’s instructions. Inhibition rate (%) was calculated as follows: Inhibition rate (%) = 100% − [(No. of live parasites in treated sample/No. of live parasites in untreated control) × 100%].
To evaluate the inhibitory effects of CsA, DHCsA-d, or SSG on intracellular amastigotes, we infected macrophages of a murine macrophage stable cell line (RAW 264.7) (Jennio, Guangzhou, China) with logarithmic phase promastigotes. RAW 264.7 cells (5.0 × 105 cells/per well) were plated on round glass coverslips in 24-well plates and allowed to adhere to the slides for 24 h at 37 °C, 5% CO2, in PRMI 1640 medium (Gibco, Franklin, TN, USA) supplemented with 10% FBS (Gibco). Adherent macrophages were infected with L. donovani promastigotes, at a macrophages-to-parasite ratio of 1:20 for 6 h at 37 °C, 5% CO2. Next, the non-infected parasites were removed by washing three times with PBS, and the infected macrophages were incubated in 37 °C in 5% CO2 with PRMI 1640 medium and 10% FBS without drugs for 24 h. The medium was then removed and different concentrations of CsA (3, 6, 10, 15, 20 μM), DHCsA-d (3, 6, 10, 15, 20 μM) or SSG (5, 10, 25, 50, 90 μM) dissolved in fresh medium were added, and the coverslips were incubated for 2 days. At 24 and 48 h, the glass coverslips were fixed in methanol (Solarbio, Beijing, China) and stained with Wright’s stain (Solarbio). The numbers of parasites were determined using light microscopy by counting at least 200 cells per slide. The results are expressed as means of three independent experiments. The 50% inhibitory concentration (IC50) was calculated for promastigotes and intracellular amastigotes by fitting the values to a non-linear curve analysis.
CsA, DHCsA-d, or SSG-treated control promastigotes and intracellular amastigotes within the macrophages of RAW 264.7 cell line were fixed in 2.5% glutaraldehyde in 0.1 M cacodylate buffer (pH 7.2) and post-fixed in a solution containing 1% OsO4, 1.25% potassium ferrocyanide and 0.1 M cacodylate buffer, pH 7.2. Next, the cells were dehydrated in acetone and embedded in epoxy resin. Stained with lead citrate and observed under a Hitachi HT7700 transmission electron microscope.
Production of polyclonal antibody of LdCyPA and western blotting
Polyclonal antibodies against LdCyPA were obtained to monitor protein expression. Representative peptides of LdCyPA were analyzed through two predictors for B cells, BEPIPRED and BCPRED12. Among these, 8 peptides were found to be highly immunogenic. The LdCyPA gene was amplified by PCR (forward primer: 5′-CGC CGA ATT CAT GTC TTA CAC GCC GCA CTA CCC CG-3′; reverse primer: 5′-CCG GTC GAC TTA AAG CTG TCC GCA GGC AGC CAC G-3′) and cloned into pET28a (Promega, Madison, WI, USA) for sequencing and expressing proteins. Polyclonal antiserum was produced in New Zealand white rabbits. The rabbits were immunized with Freund’s adjuvant (Sigma-Aldrich), containing 1500 μg of LdCyPA peptide, on days 0, 15 and 30. The rabbits received three subcutaneous injections, the first in complete Freund’s adjuvant and later two in incomplete Freund’s adjuvant. Serum was obtained and antibody titers were estimated by ELISA on 25 and 42 days after the last injection.
Promastigotes, intracellular amastigotes and RAW 264.7 cells were co-cultured with the three compounds, CsA, DHCsA-d, or SSG for 48 h. Promastigotes were treated with CsA (16 μM), DHCsA-d (12 μM), or SSG (20 μM); intracellular amastigotes and RAW 264.7 cells were treated with CsA (10 μM), DHCsA-d (5 μM), or SSG (9 μM). These cells were then lysed with a protein lysis buffer supplemented with protease and phosphatase inhibitors and the protein concentration was determined by the BCA Kit (Beyotime). The extracted proteins were denatured for 5 min at 100 °C after adding appropriate amounts of loading buffer. Approximately 40 to 50 μg of proteins was loaded in each lane of a 12% polyacrylamide gel (Beyotime). Proteins were separated at 120 V until the dye front reached the bottom of the gel, followed by transfer of the gels to polyvinylidene fluoride (PVDF) membranes (EMD, MA, USA) in transfer buffer (25 mM Tris-HCl, 192 mM glycine, 20% methanol, 0.02% SDS, pH 8.3) and run at 200 mA for 60 min. The membranes were then soaked in a blocking buffer (1 × PBS, 0.1% Tween 20) and supplemented with 1% bovine serum albumin (Sigma-Aldrich) for 2 h, before incubating overnight at 4 °C individually with LdCyPA polyclonal antibody, CyPA antibody (Affinity, Dublin, OH, USA) and α-tubulin antibody (Affinity) at appropriate dilutions. All the primary antibodies were used at a 1:4000 dilution and horseradish peroxidase-conjugated anti-rabbit immunoglobulin secondary antibodies (Affinity) were used at a 1:5000 dilution. The PVDF membranes were visualized with an enhanced chemiluminescence western blotting detection kit (Beyotime) and the protein bands were analyzed by densitometric studies using ImageJ software.
Quantification of cytokines, NO and H2O2
Mouse RAW 264.7 macrophages (5.0 × 105 cells/per well), adhered for 24 h at 37 °C, 5% CO2, in PRMI 1640 medium supplemented with 10% FBS were infected with promastigotes at a macrophages-to-parasite ratio of 1:20 for 6 h at 37 °C, 5% CO2, and subsequently the non-infected parasites were removed by washing three times with PBS. Infected macrophages were incubated in PRMI 1640 medium and 10% FBS at 37 °C, 5% CO2, without drugs for 24 h. Next, the medium was removed and CsA (10 μM), DHCsA-d (5 μM), or SSG (9 μM) (concentrations showing IC50 for intercellular amastigotes in this study) were added using fresh medium. The cells were further incubated for 3 days, and the medium supernatants were retrieved at 24, 48 and 72 h. Subsequently, the cytokines IL-12, IL-10, IL-4, IFN-γ and TNF-α were measured utilizing the BD OpitELA ELISA Kit (BD). NO and H2O2 concentrations in the supernatants were detected by nitric oxide and hydrogen peroxide assay kits (Beyotime), respectively.
Cytotoxicity effects of CsA, DHCsA-d, or SSG against murine macrophages (RAW 264.7) were assessed by using the Cell Counting Kit-8 (KeyGEN, Shanghai, China). Murine macrophages were cultivated in a 96-well plate using PRIM 1640 medium containing 10% FBS and maintained at 37 °C, 5% CO2, for 24 h. Next, different concentrations of the drugs (7, 10, 20, 50 and 100 μM for CsA and DHCsA-d; 60, 75, 90, 105 and 120 μM for SSG) were added. The cytotoxicity was measured at 24 and 48 h following a standard protocol.
All experiments were carried out in triplicates and repeated at least three times and the figures shown are representative of these experiments. IC50 were calculated according to a nonlinear regression using a log inhibitor-versus response equation with 95% confidence intervals in the GraphPad Prism 6.0 software. The data were analyzed using Student’s t-test for comparison of two groups and data values were expressed as the mean ± standard deviation (SD). Significant differences were determined and designated with asterisks as follows: *P < 0.05; **P < 0.01; ***P < 0.001 and ****P < 0.0001.
We treated promastigotes with different concentrations of CsA, DHCsA-d, or SSG for 24 and 48 h; this was followed by flow cytometry using annexin V-FITC and PI labeling. All the three drugs could inhibit promastigotes at 24 h (Fig. 1a) and their inhibitory effect was enhanced over a period of time (Fig. 1b). The inhibition rates were calculated (Fig. 1c, d). Intracellular amastigotes were treated with different concentrations of CsA, DHCsA-d, or SSG for 24 and 48 h followed by microscopy to calculate inhibition rates (Fig. 2i, j). The results of Wright’s staining suggested that compared to the numbers of untreated amastigotes (Fig. 2a, b), the numbers of DHCsA-d-treated or SSG-treated intracellular amastigotes were reduced after 24 h of treatment (Fig. 2e, g) and were basically absent after 48 h of treatment (Fig. 2f, h), leaving several different sizes of parasitophorous vacuoles in the cells. Interestingly, on the contrary, the number of intracellular amastigotes was significantly increased in CsA-treated cells after a 24 h (Fig. 2c) and 48 h (Fig. 2d) treatment compared with that in the control group cells.
Based on the inhibitory effect of different concentrations of the drugs assessed, IC50 values of these three drugs were calculated (Table 1). The IC50 values of DHCsA-d-treated promastigotes were 21.24 μM (24 h) and 12.14 μM (48 h). Likewise, DHCsA-d had a striking inhibitory effect on the growth of intercellular amastigotes. The IC50 values of DHCsA-d-treated amastigotes were 5.23 μM and 4.84 μM at 24 and 48 h, respectively. CsA was also active against promastigotes, showing an IC50 value of 23.44 μM at 24 h and 15.88 μM at 48 h. The IC50 value of CsA towards intercellular amastigotes was not determined because we found that the number of amastigotes in the CsA-treated group was increased compared with that in the control group. The SSG group showed IC50 values of 32.33 μM (24 h) and 20.23 μM (48 h) for promastigotes and 9.51 μM (24 h) and 8.27 μM (48 h) for amastigotes.
Drugs altered mitochondrial ultrastructure
CsA, DHCsA-d, or SSG induced significant morphological changes in promastigotes, including increased aggregate formation, oval cell shape and shortened and motionless flagellae (Fig. 3b–d). The ultrastructure of the main organelles of L. donovani was also significantly altered after treatment with CsA, DHCsA-d, or SSG, especially that of the mitochondria, which appeared completely disorganized (Fig. 3b–d). As shown in Fig. 3a, the control promastigotes presented normal ultrastructure for mitochondria and nuclei. Moreover, there was an abnormal increase in the number of flagellae in DHCsA-d-treated promastigotes (Fig. 3c).
The untreated intracellular amastigotes presented normal ultrastructure for nuclei and mitochondria (Fig. 4a). The mitochondria of intracellular amastigotes treated with DHCsA-d or SSG appeared disintegrated (Fig. 4c, d). Almost half of the DHCsA-d-treated intracellular amastigotes were degraded in parasitophorous vacuoles (Fig. 4c). CsA-treated intracellular amastigotes remained unchanged, unlike the CsA-treated promastigotes, which did not show significant changes as compared to the untreated group (Fig. 4b).
The effect of CsA, DHCsA-d, or SSG on cytokine, NO and H2O2 production
CsA, DHCsA-d, or SSG were incubated with L. donovani non-infected and infected macrophages. The supernatants of the medium were assayed to quantify pro-inflammatory cytokines (IL-12, IFN-γ and TNF-α), which are crucial for the successful treatment of VL and anti-inflammatory cytokines (IL-10 and IL-4), which participate in the exacerbation of the disease. The levels of cytokines were evaluated by ELISA. IL-12, IFN-γ and TNF-α all showed significant downregulation after infection (Fig. 5a–c). Leishmania donovani are found to be sensitive to DHCsA-d and SSG, thus the DHCsA-d and SSG treatments resulted in significant increases of IL-12, IFN-γ and TNF-α in L. donovani infected cells on the 24 h, 48 h and 72 h. However, the levels of these three cytokines did not change significantly in L. donovani-infected cells in the CsA-treated group compared to those in the untreated group.
The tendencies of variation of the cytokines IL-10 and IL-4 and NO and H2O2 production were identical. IL-10, IL-4, NO and H2O2 production showed significant enhancement after infection (Fig. 5d–g) but was observed to be significantly decreased in DHCSA-d and SSG- treated L. donovani at 24 h, 48 h and 72 h. However, the levels of IL-10, IL-4, NO and H2O2 did not change significantly in L. donovani infected cells in the CsA-treated group compared to those in the untreated group. Furthermore, the levels of all the five cytokines and NO and H2O2 production decreased over a period of time in all groups after treatment. The results of statistical tests were calculated (Table 2).
Preparation of LdCyPA antibody
The LdCyPA gene was successfully amplified by PCR and ligated into the plasmid pET-28a. The construction of the recombinant plasmid was verified by double enzyme digestion. The recombinant pET-28a vector was then transferred into BL21 cells to express the fusion protein, which was purified using Ni-NTA agarose affinity chromatography and verified by the sodium dodecyl sulfate polyacrylamide gel electrophoresis (Fig. 6a, b). Further, western blotting demonstrated that a purified LdCyPA protein was obtained (Fig. 6c). The concentration of the LdCyPA protein was 3.87 mg/ml, as estimated by the BCA method. Serum samples of rabbits immunized with LdCyPA were collected for detection of the titers on 25 and 42 days. Since the titers were greater than 1:50,000 according to ELISA, the sera of these rabbits were further purified to obtain specific LdCyPA antibodies.
The expression of CyPA and LdCyPA after drug inhibition
The expression of LdCyPA in promastigotes (t(4) = 11.45, P = 0.0003) and intracellular amastigotes (t(4) = 18.85, P < 0.0001) treated with CsA and the expression of CyPA in RAW 264.7 cells (t(4) = 12.95, P = 0.0002) treated with CsA were found to be significantly downregulated compared to those in the untreated cells (Fig. 7a–f). However, no significant changes were found in the expression levels of LdCyPA in promastigotes (t(4) = 2.076, P = 0.1065; t(4) = 1.45, P = 0.2206) and intracellular amastigotes (t(4) = 0.1112, P = 0.9168; t(4) = 1.131, P = 0.3213) and CyPA in RAW 264.7 cells (t(4) = 1.862, P = 0.1361; t(4) = 0.2635, P = 0.8052) treated with DHCsA-d or SSG compared to those in the untreated cells (Fig. 7a–f). Densitometric analysis results showed lower LdCyPA levels in promastigotes and amastigotes treated with CsA than in those treated with DHCsA-d or SSG (Fig. 7d, e) and lower CyPA levels were seen in RAW 264.7 cell co-cultured with CsA than those co-cultured with DHCsA-d or SSG (Fig. 7f).
Dihydrocyclosporin A induced high cytotoxicity in RAW264.7 cells
The safety profile of CsA, DHCsA-d, or SSG was examined using a mammalian cytotoxicity test using RAW 264.7 cells. CsA and DHCsA-d demonstrated cytotoxicity towards macrophages, showing 50% cytotoxic concentration (CC50) values of 15.91 μM (CsA, 24 h), 12.65 μM (CsA, 48 h), 7.98 μM (DHCsA-d, 24 h) and 6.65 μM (DHCsA-d, 48 h); by contrast, SSG exhibited a CC50 value > 120 μM (Table 3).
VL is potentially fatal to patients if left untreated. Because it causes severe immunosuppression, it makes patients more susceptible to secondary microbial infections . Due to the drug resistance, high cost, toxic side effects, and lengthy treatment regimens of pentavalent antimonials, it is necessary to find an alternative therapeutic drug for VL. As mentioned above, CsA and its non-immunosuppressive derivatives were considered to be potential therapeutic drugs to treat VL. However, whether CsA and its derivatives can be used as therapeutic drugs for VL has been controversial for many years.
In this study, the inhibitory effects of CsA and its derivative DHCsA-d on promastigotes and intracellular amastigotes of L. donovani were assessed. The number of intracellular amastigotes decreased significantly compared to that in the untreated group after administration of DHCsA-d or SSG. However, the number of intracellular amastigotes distinctly increased after the administration of CsA. These results indicated that CsA and DHCsA-d had anti-leishmanial effects on promastigotes, while CsA was found to promote the infection of intracellular amastigotes.
The role of CsA in promoting intracellular amastigote infection was confirmed by assessing morphological observation and cytokine expression levels in this study. According to ultrastructure observations, after treatment with DHCsA-d or SSG, there were obvious changes in the mitochondria of promastigotes and amastigotes. The mitochondria were completely disorganized; this result was similar to the findings regarding ultrastructural changes in the mitochondria of L. amazonensis treated with itraconazole and ravuconazole [26, 27]. However, no obvious changes in mitochondria were observed after treatment with CsA.
Appropriate activation of macrophages, which are the major effector cells responsible for elimination of leishmania, is crucial for eliminating intracellular Leishmania . Therefore, the effects of three pro-inflammatory cytokines (IL-12, IFN-γ and TNF-α), which are crucial for the successful treatment of VL and anti-inflammatory cytokines (IL-4 and IL-10), which participate in the exacerbation of the disease, secreted by macrophages, were evaluated by ELISA in this study. We found that the levels of IL-4 and IL-10 were significantly increased, while those of IL-12, IFN-γ and TNF-α were significantly decreased after phagocytosis of L. donovani by macrophages. These results are supported by the cytokine expression in VL patients who were infected with L. donovani . High levels of IL-10 were found in the serum of these VL patients, which could inhibit the activity of pro-inflammatory cytokines, such as IFN-γ and TNF-α . Macrophages produce IL-12 to promote a Th1 response during leishmanial infection, which protects the host and controls parasite replication [30, 31]. Meanwhile, TNF-α and IFN-γ, implicated to be involved in the activation of macrophages, were also observed to play a role in preventing parasite replication . Previous studies also verified that drugs which have inhibitory effects on L. donovani, could decrease IL-10 and IL-4 in VL mice [4, 33, 34]. In this study, the reduction of parasite burden was supported by the increase of IL-12, IFN-γ and TNF-α and decrease of IL-4 and IL-10 after DHCsA-d or SSG treatments. On the contrary, the levels of IL-12, IFN-γ and TNF-α decreased and IL-4 and IL-10 increased after CsA treatment compared with those of the untreated group.
In the first few hours of leishmanial infection within macrophages, the most effective anti-parasitic response of the macrophages is the production of reactive oxygen species (ROS) and reactive nitrogen species (RNS) [35, 36]. The two major reactive species in macrophages are superoxide (O2−) and nitric oxide (NO) [37, 38]. It is observed that if drugs have ideal anti-parasitic effects, the NO and H2O2 productions of leishmania-infected macrophages decrease [4, 39]. In our research, elevated levels of NO and H2O2 were found in leishmania-infected macrophages and a strong inhibition of NO and H2O2 metabolites was observed upon treatment with DHCsA-d or SSG. However, an increase of these metabolites was observed after treatment with CsA. Meissner et al.  also found that CsA did not rely on reactive nitrogen to kill L. major by macrophages and the NO production was also not increased after CsA treatment.
Cyclophilin A (CyPA), which possesses a peptidylprolyl isomerase (PPIase) activity, is an important member of a highly conserved family of human multi-functional proteins called cyclophilins (CyPs) [16, 17]. CyPA, having an immunosuppressive action, is characterized by the binding of cyclic peptide inhibitor, CsA, which inhibits protein phosphatase calcineurin and T cell-mediated immunity . Parasite cyclophilins are also known to be potential drug targets, because the immunosuppressive drug CsA can be potentially used as an antiparasitic drug against Leishmania tropica , Schistosoma mansoni  and Plasmodium falciparum . Trypanosoma cruzi cyclophilin (TcCyP19) is suggested to play a protective role in the survival of the infected tissue and allow parasite persistence . The Leishmania cyclophilin of 19 kDa, LdCyPA, has a 79–81% protein sequence identity with the TcCyP19 . In this study, western blotting showed a decreased expression of CyPA and LdCyPA after CsA treatment, while that of DHCsA-d or SSG groups showed no significant changes. These results confirmed observations in a previous study demonstrating that cell CyPA can inhibit the immunity of macrophages by binding to CsA and that LdCyPA can promote the intracellular viability and proliferation of leishmania by binding to CsA. According to the above results, since CsA is not shown to have an inhibitory effect on intracellular amastigotes, we believe that CsA should not be recommended for VL treatment.
DHCsA-d had an excellent inhibitory effect on both promastigotes and intracellular amastigotes and did not inhibit the immunological effects of macrophages or promote leishmania infection. Unfortunately, the CC50 of DHCsA-d was only 7.98 μM (24 h) and 6.65 μM (48 h) in this study, suggesting its high cytotoxicity. Therefore, DHCsA-d is also not recommended for VL treatment. This study demonstrated that CsA and DHCsA-d might not be ideal antileishmanial agents due to various limitations, which may provide a reference for subsequent researches.
The results of our study have resolved the dispute regarding the efficacy of CsA and DHCsA-d for VL treatment. CsA did not show a significant inhibitory effect on the intracellular amastigotes of L. donovani. DHCsA-d significantly inhibited promastigotes and intracellular amastigotes, but it was found to be highly cytotoxic. We believe that CsA and DHCsA-d should not be recommended as antileishmanial drugs. Research towards new therapeutic drugs for VL has a long way to go and further studies are required to develop appropriate anti-leishmanial drugs.
Availability of data and materials
The datasets supporting the conclusions of this article are included within the article.
Leishmania donovani Cyclophilin A
- SbV :
- IC50 :
50% inhibitory concentration
- CC50 :
50% cytotoxic concentration
Enzyme-linked immunosorbent assay
Alvar J, Velez ID, Bern C, Herrero M, Desjeux P, Cano J, et al. Leishmaniasis worldwide and global estimates of its incidence. PLoS ONE. 2012;7:e35671.
Lun ZR, Wu MS, Chen YF, Wang JY, Zhou XN, Liao LF, et al. Visceral leishmaniasis in China: an endemic disease under control. Clin Microbiol Rev. 2015;28:987–1004.
Guerin PJ, Olliaro P, Sundar S, Boelaert M, Croft SL, Desjeux P, et al. Visceral leishmaniasis: current status of control, diagnosis and treatment and a proposed research and development agenda. Lancet Infect Dis. 2002;2:494–501.
Chauhan K, Kaur G, Kaur S. Activity of rutin, a potent flavonoid against SSG-sensitive and -resistant Leishmania donovani parasites in experimental leishmaniasis. Int Immunopharmacol. 2018;64:372–85.
Bell A, Roberts HC, Chappell LH. The antiparasite effects of cyclosporin A: possible drug targets and clinical applications. Gen Pharmacol. 1996;27:963–71.
Chappell LH, Wastling JM. Cyclosporin A: antiparasite drug, modulator of the host-parasite relationship and immunosuppressant. Parasitology. 1992;105(Suppl.):25–40.
Solbach W, Forberg K, Kammerer E, Bogdan C, Rollinghoff M. Suppressive effect of cyclosporin A on the development of Leishmania tropica-induced lesions in genetically susceptible BALB/c mice. J Immunol. 1986;137:702–7.
Solbach W, Forberg K, Rollinghoff M. Effect of T-lymphocyte suppression on the parasite burden in Leishmania major-infected, genetically susceptible BALB/c mice. Infect Immun. 1986;54:909–12.
Hoerauf A, Rascher C, Bang R, Pahl A, Solbach W, Brune K, et al. Host-cell cyclophilin is important for the intracellular replication of Leishmania major. Mol Microbiol. 1997;24:421–9.
Eldaw A, Sequeira RP, Eldirdiri AB. A preliminary observation on in vitro inhibitory effect of cyclosporin-A upon growth of Leishmania tropica promastigotes. J Egypt Soc Parasitol. 1989;19:301–5.
Yau WL, Blisnick T, Taly JF, Helmer-Citterich M, Schiene-Fischer C, Leclercq O, et al. Cyclosporin A treatment of Leishmania donovani reveals stage-specific functions of cyclophilins in parasite proliferation and viability. PLoS Negl Trop Dis. 2010;4:e729.
Merelli M, Quartuccio L, Bassetti M, Pecori D, Gandolfo S, Avellini C, et al. Efficacy of intravenous cyclosporine in a case of cytophagic histiocytic panniculitis complicated by haemophagocytic syndrome after visceral leishmania infection. Clin Exp Rheumatol. 2015;33:906–9.
Adinolfi LE, Bonventre PF. Cyclosporin A treatment converts Leishmania donovani-infected C57BL/10 (curing) mice to a noncuring phenotype. Infect Immun. 1990;58:3151–3.
Olivier M, Proulx C, Tanner CE. Importance of lymphokines in the control of multiplication and dispersion of Leishmania donovani within liver macrophages of resistant and susceptible mice. J Parasitol. 1989;75:720–7.
Olivier M, Tanner CE. The effect of cyclosporin A in murine visceral leishmaniasis. Trop Med Parasitol. 1989;40:32–8.
Roberts HC, Sternberg JM, Chappell LH. Characterization of calcineurin from Hymenolepis microstoma and H. diminuta and its interaction with cyclosporin A. Parasitology. 1997;114:279–83.
Xue C, Sowden MP, Berk BC. Extracellular and intracellular cyclophilin A, native and post-translationally modified, show diverse and specific pathological roles in diseases. Arterioscler Thromb Vasc Biol. 2018;35:986–93.
Peacock CS, Seeger K, Harris D, Murphy L, Ruiz JC, Quail MA, et al. Comparative genomic analysis of three Leishmania species that cause diverse human disease. Nat Genet. 2007;39:839–47.
Rogers MB, Hilley JD, Dickens NJ, Wilkes J, Bates PA, Depledge DP, et al. Chromosome and gene copy number variation allow major structural change between species and strains of Leishmania. Genome Res. 2011;21:2129–42.
Perrone AE, Milduberger N, Fuchs AG, Bustos PL, Bua J. A functional analysis of the cyclophilin repertoire in the protozoan parasite Trypanosoma cruzi. Biomolecules. 2018;8:E132.
Meier GP, Park SB, Yee GC, Gmur DJ. Isolation and identification of a novel human metabolite of cyclosporin A: dihydro-CsA M17. Drug Metab Dispos. 1990;18:68–71.
Chappell LH, Thomson AW, Barker GC, Smith SW. Dosage, timing, and route of administration of cyclosporin A and nonimmunosuppressive derivatives of dihydrocyclosporin A and cyclosporin C against Schistosoma mansoni in vivo and in vitro. Antimicrob Agents Chemother. 1987;31:1567–71.
Veronica J, Chandrasekaran S, Dayakar A, Devender M, Prajapati VK, Sundar S, et al. Iron superoxide dismutase contributes to miltefosine resistance in Leishmania donovani. FEBS J. 2019;286:3488–503.
Vermeersch M, da Luz RI, Tote K, Timmermans JP, Cos P, Maes L. In vitro susceptibilities of Leishmania donovani promastigote and amastigote stages to antileishmanial reference drugs: practical relevance of stage-specific differences. Antimicrob Agents Chemother. 2009;53:3855–9.
ter Horst R, Collin SM, Ritmeijer K, Bogale A, Davidson RN. Concordant HIV infection and visceral leishmaniasis in Ethiopia: the influence of antiretroviral treatment and other factors on outcome. Clin Infect Dis. 2008;46:1702–9.
Teixeira de Macedo Silva S, Visbal G, Lima Prado Godinho J, Urbina JA, de Souza W, Cola Fernandes Rodrigues J. In vitro antileishmanial activity of ravuconazole, a triazole antifungal drug, as a potential treatment for leishmaniasis. J Antimicrob Chemother. 2018;73:2360–73.
de Macedo-Silva ST, Urbina JA, de Souza W, Rodrigues JC. In vitro activity of the antifungal azoles itraconazole and posaconazole against Leishmania amazonensis. PLoS ONE. 2013;8:e83247.
Mukbel RM, Patten C Jr, Gibson K, Ghosh M, Petersen C, Jones DE. Macrophage killing of Leishmania amazonensis amastigotes requires both nitric oxide and superoxide. Am J Trop Med Hyg. 2007;76:669–75.
Faleiro RJ, Kumar R, Hafner LM, Engwerda CR. Immune regulation during chronic visceral leishmaniasis. PLoS Negl Trop Dis. 2014;8:e2914.
Hernandez-Pando R, Orozco H, Arriaga K, Sampieri A, Larriva-Sahd J, Madrid-Marina V. Analysis of the local kinetics and localization of interleukin-1 alpha, tumour necrosis factor-alpha and transforming growth factor-beta, during the course of experimental pulmonary tuberculosis. Immunology. 1997;90:607–17.
Watford WT, Hissong BD, Bream JH, Kanno Y, Muul L, O’Shea JJ. Signaling by IL-12 and IL-23 and the immunoregulatory roles of STAT4. Immunol Rev. 2004;202:139–56.
Rossi M, Fasel N. How to master the host immune system? Leishmania parasites have the solutions! Int Immunol. 2018;30:103–11.
Kaur R, Kaur S. Evaluation of in vitro and in vivo antileishmanial potential of bergenin rich Bergenia ligulata (Wall.) Engl. root extract against visceral leishmaniasis in inbred BALB/c mice through immunomodulation. J Tradit Complement Med. 2018;8:251–60.
Lapara NJ 3rd, Kelly BL. Suppression of LPS-induced inflammatory responses in macrophages infected with Leishmania. J Inflamm. 2010;7:8.
Iles KE, Forman HJ. Macrophage signaling and respiratory burst. Immunol Res. 2002;26:95–105.
Fang FC. Antimicrobial reactive oxygen and nitrogen species: concepts and controversies. Nat Rev Microbiol. 2004;2:820–32.
Panday A, Sahoo MK, Osorio D, Batra S. NADPH oxidases: an overview from structure to innate immunity-associated pathologies. Cell Mol Immunol. 2015;12:5–23.
Aktan F. iNOS-mediated nitric oxide production and its regulation. Life Sci. 2004;75:639–53.
Pereira AV, de Barros G, Pinto EG, Tempone AG, Orsi Rde O, Dos Santos LD, et al. Melittin induces in vitro death of Leishmania (Leishmania) infantum by triggering the cellular innate immune response. J Venom Anim Toxins Incl Trop Dis. 2016;22:1.
Meissner U, Juttner S, Rollinghoff M, Gessner A. Cyclosporin A-mediated killing of Leishmania major by macrophages is independent of reactive nitrogen and endogenous TNF-alpha and is not inhibited by IL-10 and 13. Parasitol Res. 2003;89:221–7.
Bell A, Wernli B, Franklin RM. Roles of peptidyl-prolyl cis-trans isomerase and calcineurin in the mechanisms of antimalarial action of cyclosporin A, FK506, and rapamycin. Biochem Pharmacol. 1994;48:495–503.
Bua J, Aslund L, Pereyra N, Garcia GA, Bontempi EJ, Ruiz AM. Characterisation of a cyclophilin isoform in Trypanosoma cruzi. FEMS Microbiol Lett. 2001;200:43–7.
This study was supported by the National Natural Science Foundation of China to JL (31802184), JC (81672048) and DC (31572240, 31872959).
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This study was approved by the Sichuan University Medical Ethics Committee (Approval Number: K2018056). All animal experimental procedures were performed according to the regulations laid down by the Administration of Affairs Concerning Experimental Animals approved by the State Council of People’s Republic of China.
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Zheng, ZW., Li, J., Chen, H. et al. Evaluation of in vitro antileishmanial efficacy of cyclosporin A and its non-immunosuppressive derivative, dihydrocyclosporin A. Parasites Vectors 13, 94 (2020). https://doi.org/10.1186/s13071-020-3958-x
- Cyclosporine A
- Dihydrocyclosporin A
- Cyclophilin A
- Visceral leishmaniasis