The protozoan parasite Cryptosporidium parvum is responsible for significant disease burden among children in developing countries. In addition Cryptosporidiosis can result in chronic and life-threatening enteritis in AIDS patients, and the currently available drugs lack efficacy in treating these severe conditions. The discovery and development of novel anti-cryptosporidial therapeutics has been hampered by the poor experimental tractability of this pathogen. While the genome sequencing effort has identified several intriguing new targets including a unique inosine monophosphate dehydrogenase (IMPDH), pursuing these targets and testing inhibitors has been frustratingly difficult. Here we have developed a pipeline of tools to accelerate the in vivo screening of inhibitors of C. parvum IMPDH. We have genetically engineered the related parasite Toxoplasma gondii to serve as a model of C. parvum infection as the first screen. This assay provides crucial target validation and a large signal window that is currently not possible in assays involving C. parvum. To further develop compounds that pass this first filter, we established a fluorescence-based assay of host cell proliferation, and a C. parvum growth assay that utilizes automated high-content imaging analysis for enhanced throughput. We have used these assays to evaluate C. parvum IMPDH inhibitors emerging from our ongoing medicinal chemistry effort and have identified a subset of 1,2, 3-triazole ethers that exhibit excellent in vivo selectivity in the T. gondii model and improved anti-cryptosporidial activity.
Gastrointestinal diseases remain the largest threat to the health of infants and small children in environments with low income and poor sanitation. While acute diarrheal disease claims numerous lives, chronic or recurrent forms can result in stunting of physical and intellectual growth in an even larger number of children. The aetiology of diarrheal disease in children is complex, involving a large group of viral, bacterial, protozoan and metazoan pathogens. Among these the protozoan parasites, Cryptosporidium parum and hominis are epidemiologically important pathogens [1], [2]. Cryptosporidium causes acute self-limiting gastrointestinal disease in healthy individuals. Immunity is slow to develop and the disease can be recurrent and protracted in malnourished children [3]–[6]. Malnourished children are not only more susceptible to severe cryptosporidiosis, but the disease itself is an important contributing factor to malnutrition [7]. In immunocompromised individuals like those suffering from AIDS, cryptosporidiosis is a chronic and life-threatening disease [8]. The persistent and resilient nature of the infective oocyst stage in drinking and recreational water poses significant challenges for controlling transmission even in industrialised nations. No vaccines exist, and the currently available drugs are inadequate. The more widely used drugs paromomycin and azithromycin are unreliable and the efficacy of nitazoxanide, which recently received FDA approval, is dependent upon a robust immune response [9]. The options in particular for the treatment of chronic AIDS-related cryptosporidiosis are severely limited [10] and there is an overall urgent need for new chemotherapy. The sequencing of the genomes of Cryptosporidium parvum and hominis revealed a highly streamlined anabolic metabolism with potential choke points that might be exploited in drug design [11], [12]. One such vulnerability lies in the pathway that supplies purine nucleotides for the synthesis of DNA and RNA. Like all protozoan parasites, Cryptosporidium is incapable of de novo purine synthesis and relies on salvage of purines from the host. While many parasites, including the related Apicomplexa Toxoplasma and Plasmodium, use hypoxanthine-xanthine-guanine phosphoribosyltransferase (HXGPRT, Figure 1) to salvage a broad range of purine bases this enzyme is missing in Cryptosporidium [12], [13]. Instead, Cryptosporidium relies solely on the salvage of adenosine to provide both adenine and guanine nucleotides. This simplified pathway is initiated by adenosine kinase and critically depends on the activity of inosine monophosphate dehydrogenase (CpIMPDH). Surprisingly, the CpIMPDH gene appears to have been acquired through lateral gene transfer from an ε-proteobacterium [13], [14]. Detailed kinetic analysis of this prokaryote-like enzyme demonstrated that CpIMPDH is very different from its human homologs [13], [15]. The “drugability” of IMPDH is well established as inhibitors of human IMPDHs have been used clinically as immunosuppressants as well as for the treatment of viral infections and cancer [16]–[18]. Taken together, these observations suggest that CpIMPDH is a promising therapeutic target for cryptosporidiosis [13]–[15], [19]. We have recently discovered several new classes of selective inhibitors of CpIMPDH in a high throughput screen [20]. Extensive medicinal chemistry optimization has produced nanomolar inhibitors with greater than 103-fold selectivity for CpIMPDH over the human enzymes [21], [22]. Further elaboration of these compounds requires a rapid and reliable assay to evaluate their anti-parasitic activity. The screening of compounds against C. parvum has proven challenging and the main roadblock in our drug development program. This is partly because the parasite cannot be cultured continuously in tissue culture. Although several growth assays have been developed, including real-time PCR protocols [23]–[28], immunoassays [29], [30], and image analysis routines [31], these assays are labour intensive and expensive, or are not amenable to higher throughput. The scarcity of experimental tools for C. parvum also makes it difficult to investigate the mechanism of inhibitor action. In this study we describe an assay pipeline to evaluate the anti-cryptosporidial activity of CpIMPDH inhibitors in tissue culture models. We have genetically engineered the related apicomplexan parasite T. gondii to mirror the purine pathway of Cryptosporidium and to depend on CpIMPDH for survival. This system provides a rapid assessment of anti-parasitic potential and a quantitative read of target specificity. To further evaluate if anti-cryptosporidial activity arises from off-target effects on the host cell, we devised a simple and highly sensitive host cell growth assay using an HCT-8 line engineered to express a yellow fluorescent protein. Lastly, we have developed a new high-content imaging assay to measure C. parvum proliferation directly. We have utilized these assays to probe the structure-activity relationship for a series of CpIMPDH inhibitors [20], [22]. We discovered five compounds that exhibited potency and selectivity in the T. gondii model, including two that show sub-micromolar anti-cryptosporidial activity.
Cosmid TOXOU05 [32] was selected using the ToxoDB database [33]. The 42. 2 Kb genomic DNA insert of TOXTOU05 spans the TgIMPDH open reading frame with 14. 3 Kb and 22. 7 Kb of flanking sequence at the 5′ and 3′ ends respectively. A schematic overview of the cosmid modification steps is shown in Figure S1 [34]. Initial cosmid amplification was performed in E. coli strain XL1Blue using LB containing 10 µg/ml kanamycin. The QIAprep Spin Miniprep kit (QIAGEN) was used with slight modification to the standard protocol for cosmid purification. Following the addition of buffer P3 and centrifugation cosmid DNA was directly precipitated from the supernatant using 0. 7 volumes of isopropanol. Cosmid DNA (200 ng) was introduced into the E. coli EL250 strain [35] by electroporation (ECM 630,1 mm cuvette, 1. 75 kV, 250 Ω, and 25 µF; BTX; Holliston, MA) and bacteria were propagated in LB (50 µg/ml kanamycin) and rendered electro-competent. A cassette, comprising a bacterial gentamycin selectable marker and the chloramphenicol resisftance gene flanked by the 5′ and 3′ UTRs of the T. gondii GRA1 gene (for selection in the parasite) was amplified from plasmid piCG [34] by PCR. To drive recombination between the cosmid and the GENTgraCATgra cassette to excise the IMPDH coding sequence, ∼50 bp overhangs homologous to the sequence immediately flanking the start and stop codons of the TgIMPDH gene were included in the primers (primers 973: 5- (CCTGCGTCGTTTTTGCCTCGTGGCTGTTTGGCTTGTGGGTGTCTTTCCACATACGACTCACTATAGGGCGAATTGG) and 923: 5′- GTTCCCCTTTTTATATTTCTTCTTCCGTTGCACTTCCCCAGCGAAACAAAATACGACTCACTATAGGGCGAATTGG). The PCR amplified cassette was gel purified and 200 ng were electroporated into the EL250 strain [35] bearing the TOXO05 parent cosmid and bacteria were selected using kanamycin (50 µg/ml) and gentamycin (10 µg/ml). To recycle the bacterial gentamycin selectable marker, the sequence was removed from the modified cosmid using flanking Flp sites and induction of flipase [34]. Cosmid DNA was isolated from kanamycin resistant, gentamycin sensitive clones and the removal of the gentamycin sequence was confirmed by PCR. To exchange the parasite selectable marker DHFR with the fluorescent marker YFYFP the tubYFPYFPmicGENT expression cassette was recombineered into the TOXOU05graCATgraΔIMPDH cosmid in EL250 E. coli following the method described above. The tubYFPYFPmicGENT cassette was amplified from the pYG plasmid using primers (874: 5′-GTTCCCCTTTTTATATTTCTTCTTCCGTTGCACTTCCCCAGCGAAACAAAATACGACTCACTATAGGGCGAATTGG and 875: 5′- GTCGTGGGCAGACAGCAACAGTCCAGCACTCTAGCGGCATACAGAACGATCTTCTTAGGTGGCGGTACTTGGGTC). Approximately 50 bp overhangs homologous to the sequence flanking the DHFR coding sequence were included in these primers to drive recombination to create TOXOU05CATΔIMPDHYFPYFP. Restriction enzymes HindIII, NdeI and NotI were used to confirm appropriate recombination in the final cosmid DNA preparation. T. gondii RHΔHX-CpIMPDH-5MX clone [14] was electroporated with 25 µg of circular TOXOU05CATΔIMPDHYFPYFP cosmid (Figure S1). The parasites were cultured in hTERT cells and selected under 6. 8 µg/ml chloramphenicol as described previously [36]. Chloramphenicol resistant parasite clones were PCR screened using 2 primer pairs to the graCATgra cassette and 2 primer pairs to the TgIMPDH coding sequence and a single primer pair to the tubYFPYFPmicGENT cassette. This PCR screen indicated that double-homologous recombination at the TgIMPDH locus had occurred in 2 clones. Southern blotting confirmed that double homologous recombination had occurred to replace the native TgIMPDH locus with the graCATgra expression. Probe 1 was amplified from wild-type T. gondii genomic DNA using primers 1108 (5′-CGATGTCGGGGAATCACAAGCGAGAACA) and 1109 (5′-ATGTCTTCTACGAARGCGRGAGTGGTGC). Wild-type T. gondii and T. gondii-ΔHXGPRT parasites were transfected with plasmid ptubYFPYFsagCAT [37] which drives constitutive cytoplasmic expression of two copies of the yellow fluorescent protein. Similarly, plasmid pCTR2T [38] was transfected into T. gondii-CpIMPDH resulting in constitutive cytoplasmic expression of a tandem of the tomato variant of the red fluorescent protein [39]. Fluorescent parasites were selected and cloned by cell sorting using a MoFlo Legacy instrument (Beckman Coulter, Inc). Growth of fluorescent clones was monitored in 96 well plates as previously described [37]. Briefly, fluorescence was read daily with a SpectraMax M22/M2e (Molecular Devices) plate reader (Ex 485, Em 530) for 6–7 days. For each of the three fluorescent T. gondii clones percent growth inhibition was calculated on a day within the exponential phase of growth for the purpose of determining an IC50 for each compound. T. gondii genomic DNA was extracted using the DNeasy kit (QIAGEN). 1. 0 µg of genomic DNA and 2. 5 ng of cosmid DNA was digested for 14 hours with Xho1 and separated on a 0. 9% TBE agarose gel and transferred overnight by downward transfer. The blot was hybridized over night with probe 1, which was amplified from wild-type T. gondii genomic DNA using primers 1108 (5′-CGATGTCGGGGAATCACAAGCGAGAACA) and 1109 (5′-ATGTCTTCTACGAARGCGRGAGTGGTGC). The human ileocecal adenocarcinoma epithelial cell line, HCT-8, was used to support C. parvum infection in vitro. HCT-8 cells were maintained in RPMI-1640 (Hyclone) supplemented with 10% FBS, 1 mM sodium pyruvate, 50 U/m penicillin, 50 µg/ml streptomycin, and amphotericin B. Cryptosporidium parvum oocysts were a kind gift from either Dr. Mead (Emory University) or Dr. Kissinger (University of Georgia). HCT-8 cells (2×105) were seeded into black, optical quality, thin bottom, 96-well plates (DB Falcon) to achieve a 70% confluent monolayer on the day of infection. To facilitate oocyst excystation, a procedure described by Gut et al. , was followed. Briefly, oocysts were washed twice with 1 ml of PBS (pH 7. 2), incubated for 10 minutes at 37°C in 1 ml 10 mM of HCl and then incubated for a further 10 minutes in 0. 2 ml of 200 µM sodium taurocholate at 15°C [40]. This oocyst suspension was diluted directly with DMEM (Hyclone) supplemented with 2% FBS, 50 U/ml penicillin, 50 µg/ml streptomycin, amphotericin B and 0. 2 mM L-glutamine (infection medium) to inoculate host cell monolayers at 5×105 oocysts per well. Host cell monolayers were incubated for 3 hours at 37°C prior to removal of unexcysted oocysts by aspiration and PBS wash. Infection medium was then added to the monolayers and infection was allowed to progress for 48 hours. The VVL IFA was performed in a 96-well format. Following 48 hours of culture C. parvum infected HCT-8 cells were washed with PBS and fixed with 0. 2 ml/well of 3% paraformaldehyde/PBS, permeabilized with 0. 25% Triton-X-100/PBS and blocked with 4% BSA/PBS. 0. 1 ml of fluorescein (FITC) -conjugated VVL (Vector Labs 0. 5 µg/ml) in 1% BSA/PBS was applied to wells and incubated for 45 minutes. The plates were washed twice with 200 µl/well of PBS. In the first wash DAPI was included at 0. 1 µg/ml. Finally 200 µl/well of PBS was added to the plates prior to storage at 4°C protected from light. Confocal images were acquired using a BD Biosciences Bioimager P435. The instrument was programmed to automatically change position and focus, capture montage images of 9–16,40× fields per well, and then compress and save the image files. Object finding algorithms were developed for the recognition of FITC-VVL labelled C. parvum parasites and DAPI labelled host cell nuclei using Attovision Software (BD Biosciences). Briefly, to identify FITC-VVL labelled parasites, the object finding algorithm included, a flat field correction, a polygon shape setting, a 3×3 rolling ball filter, manual pixel intensity thresholding (100 min – 4095 max), and minimum and maximum object size cut-offs of 5 pixels and 350 pixels respectively. The algorithm optimised for finding DAPI labelled host cell nuclei also included flat field correction and polygon shape setting, but applied a 25×25 rolling ball filter which is more suitable for larger objects, an automated pixel intensity threshold, minimum and maximum object size cut-offs of 200 pixels and 4000 pixels respectively, and a watershed step with an erosion factor of 8 to aid in the separation of adjacent densely packed nuclei. Note that the intensity and area size cut off exclude detection of the much smaller parasite nuclei (the human genome is three hundred times larger than the C. parvum genome). The object finding analysis steps described above recorded the number and area of objects per montage image. The output files along with a plate map file were then passed to an automated analysis pipeline (Pipeline Pilot Software, Accelrys) to calculate the mean number of parasites, the ratio of parasite number to host cell nuclei number, the mean area of parasites and host cell nuclei by well, and the percentage growth by treatment as compared to the no drug control. These analyses were exported in graphical format for each plate and the numerical values tabulated in html format. All test compounds were stored as 0. 1 M stocks in DMSO at −20°C and further diluted in DMSO to a 200× working stocks for each dilution, such that the final concentration of DMSO in the infection medium was uniformly 0. 5%. For the no drug control, DMSO alone was added to triplicate wells. As a control, a high paromomycin concentration (0. 8 mg/ml) was included on each plate in triplicate wells. Plates where this paromomycin control did not inhibit 70–80% of parasite growth were manually inspected and omitted from the final analysis. To control for potential false-positive parasite detection uninfected wells were scored in each plate and the typically low background counts were automatically subtracted from the test wells. HCT-8 cells were transfected with plasmid pmaxGFP (Amaxa) using Lipofectamine (Invitrogen). Fluorescent lines were then selected and cloned using cell sorting. Confluent monolayers of pmaxGFP expressing cells were harvested from T75 flasks and passed through a 40 µm cell strainer. Cells were seeded at 4000 cells per well into black, optical quality, thin bottom, 96-well plates. All test compounds were diluted in DMSO as described. The fluorescence was read daily with a SpectraMax M22/M2e (Molecular Devices) plate reader (Ex 485, Em 530) for 6–7 days. Percent inhibition was calculated on a day within the exponential phase of growth. All compounds were synthesized using procedures previously described [22]. Compounds A61, A64, A68 and A99 were not previously described. The NMR spectra for these compounds are included as Supplemental Materials S1.
To facilitate screening of antiparasitic activity, we constructed a T. gondii reporter parasite that mirrors the Cryptosporidium purine metabolism. Figure 1 summarizes the main differences between the two parasites in this pathway. We started with a T. gondii knockout mutant that, like C. parvum, lacks the ability to salvage xanthine and guanine via HXGPRT (T. gondii-ΔHXGPRT [41]) and introduced the CpIMPDH gene under the control of a T. gondii promoter [14]. Next the native T. gondii IMPDH gene was disrupted by replacing the entire coding sequence with a chloramphenicol acetyl transferase cassette using a new cosmid-based gene targeting approach [34]. The recombineering procedure used to modify a cosmid of the IMPDH genomic locus is summarized in Figure S1. Successful disruption of the gene was confirmed by PCR (data not shown) and Southern blotting (Figure 2A & B); note that numerous previous attempts to target this locus using smaller plasmid-based constructs failed. This manipulation created strain T. gondii-CpIMPDH-ΔHXGPRT-ΔTgIMPDH. Lastly, we introduced a fluorescent protein cassette and isolated stable transgenic parasites by cell sorting. The resulting strain is referred to as T. gondii-CpIMPDH. The growth of this new parasite can be conveniently monitored in live cultures in 96 or 384 well format using a fluorescence plate reader [37]. We similarly engineered fluorescent versions of wild-type T. gondii and T. gondii-ΔHXGPRT to serve as controls. To determine if the proliferation of T. gondii-CpIMPDH depends on CpIMPDH as designed, we performed fluorescence growth assays in the presence of varying concentrations of mycophenolic acid (MPA), comparing wild-type T. gondii, ΔHXGPRT, and CpIMPDH parasites (Figure 3A, D &G). MPA is a potent inhibitor of eukaryotic IMPDHs including TgIMPDH [17], [42] but a very poor inhibitor of prokaryotic IMPDHs. CpIMDPH is of prokaryotic origin and not inhibited by MPA at concentrations active against TgIMPDH [14], [15]. As predicted, both wild-type T. gondii and T. gondii-ΔHXGPRT are sensitive to MPA (Figure 3B & E; [13], [14], [42]), but T. gondii-CpIMPDH is resistant (Figure 3H). T. gondii-ΔHXGPRT is the most sensitive strain due to its inability to salvage xanthine/guanine from the media (EC50 = 0. 29 µM versus 2. 6 µM for the wild-type strain; Figure S2 details how an EC50 value was derived from the parasite growth curves). Supplementation of the media with xanthine (0. 33 mM) essentially renders wild-type T. gondii MPA resistant (Figure 3C; EC50≥78 µM), but has no effect on T. gondii-ΔHXGPRT (Figure 3F). In contrast, T. gondii-CpIMPDH is resistant to MPA in the absence of xanthine (EC50>65 µM), as expected given the resistance of the prokaryotic CpIMPDH (Figure 3G & I; [15]). These results demonstrate that the T. gondii model system provides a powerful tool for the evaluation of in vivo efficacy, selectivity, and specificity of CpIMPDH inhibitors. Compounds that selectively inhibit CpIMPDH will block the proliferation of T. gondii-CpIMPDH but not the wild-type and T. gondii-ΔHXGPRT strains that depend on an eukaryotic IMPDH much like the human host. In contrast, non-specific compounds that have off-target activities in the parasite or the host cell will inhibit the growth of all three strains. A general inhibitor of both prokaryotic and eukaryotic IMPDHs will block the proliferation of both T. gondii-CpIMPDH and T. gondii-ΔHXGPRT in the presence of xanthine, but will have no effect on the wild-type strain which contains HGXPRT (note that such compounds should be detected in our enzyme assays and eliminated before they reach this screen). Lastly, compounds showing poor efficacy against the T. gondii-CpIMPDH parasite may signal problems pertaining to compound uptake, stability or metabolism. Examples of these varied outcomes are discussed below. While the Toxoplasma model provides outstanding throughput and an excellent first filter it does not model all aspects of Cryptosporidium biology. A direct and efficient assay of Cryptosporidium proliferation was also needed. Fluorescent Vicia villosa lectin (VVL) has been used previously to score C. parvum growth by fluorescence microscopy [43]–[45]. VVL binds with high specificity to the C. parvum parasite, labelling sporozoites, the inner oocyst wall, and most importantly intracellular stages [40], [44], [45] but not the outer oocyst wall [46]. To accommodate the increasing number of compounds entering the SAR pipeline, we adapted the FITC-VVL immunofluorescence assay to a 96-well plate format and developed an automated imaging and analysis pipeline. Figure 4 shows an overview of the methodology. Plates are fixed, permeabilized and stained with FITC-VVL and DAPI to enumerate parasites and host cells, respectively. Using a spinning disc high-content microscope a 1. 08 mm2 area of each well, was imaged providing a robust sample typically consisting of ∼6000 host cells and ∼2000 parasite stages. The instrument is programmed to automatically move from well to well, focus and acquire 20 µm deep image stacks for the entire plate. A series of automated image compression, manipulation, and object-finding algorithms was optimized for the recognition of host cells and parasites using the DAPI and FITC channels respectively (Figure 4 A and B, see Materials and Methods for further detail). To normalize for background staining and biological variability, control wells are included for background subtraction. The massive data output is stored, managed and accessed through an Accelrys pipeline database that performs further statistical analyses and transforms raw counts into percentage growth relative to a “no drug” control. Figure 4C shows a 2-fold titration of oocysts where the highest inoculum was 5. 9×105 oocysts per well, for C. parvum growth assays 5×105 oocysts were added per well. Importantly, the algorithm can easily distinguish host and parasite, so false positives are not an issue. The inhibition of parasite proliferation by paromomycin was evaluated to demonstrate the validity of this assay. The EC50 for paromomycin measured with this assay was 97 µM (Figure 4D), which is in good agreement with several previous studies (reported EC50 values range from 65–130 µM [20], [29], [47], [48]). Perplexingly, a significant number of parasites are observed even at very high concentrations of paromomycin (∼30% relative to the “no drug” control; Figure 4A). These residual parasites may be a developmentally arrested subset of the initial inoculum (note that a similar number of parasites is detected already after 24 hours, Figure S3). Interestingly, paromomycin was also found to significantly reduce the mean parasite area in a dose responsive manner (Figure 4D), which may also suggest arrested development. The differentiation of selective antiparasitic effects from those that are a secondary consequence of a host cell effect is a critical issue in drug discovery for intracellular parasites. Cytotoxicity assays commonly reflect plasma membrane integrity, and are a crude measure of host cell effects- it is conceivable that more subtle perturbations of host cell metabolism can have an adverse effect on parasite proliferation. Therefore we sought to develop a simple and inexpensive assay of host cell growth. The human ileocecal adenocarcinoma epithelial cell line, HCT-8, which is commonly used to maintain C. parvum infection in tissue culture, was engineered to constitutively express a green fluorescent protein (GFP). Growth of this cell line was monitored daily using a fluorescent plate reader. In agreement with previous reports [49]–[51], paromomycin had negligible effects on the growth of these cells (Figure S4A). The control sodium butyrate did inhibit HCT-8 growth in a dose-dependent manner in this assay (Figure S4B), as anticipated due to previous reports of its apoptotic effects in colonic tumor cell lines [52]. These experiments validate the use of the fluorescent HCT-8 cell growth assay. The antiparasitic activities of compounds from our medicinal chemistry optimization program of compound A (identified in our initial screen [20]) were evaluated in the T. gondii model system. The structures of these compounds are shown in Figure 5 (triazoles) and Figure S5 (amides) alongside a summary of findings. Three compounds, A30, A57 and A66, do not inhibit CpIMPDH in vitro; as expected, none of these compounds selectively blocked the growth of T. gondii-CpIMPDH (Figures S5 & S6A). The remaining compounds inhibit CpIMPDH with values of IC50 ranging from 9 nM to 2. 6 µM [22]. Figure 6A shows representative data for fourteen 1,2, 3-triazole derivatives in the T. gondii model; the remaining compounds are shown in Figure S6A. With the exception of A23 and A31, all compounds inhibit the growth of the T. gondii-CpIMPDH parasite with an EC50<10 µM (Figures 6B & S6). Five of the 1,2, 3-triazole derivatives, A100, A102, A103, A109 and A110, exhibit selectivity ≥36-fold for the T. gondii-CpIMPDH parasite over wild-type T. gondii (Figure 5). Therefore the antiparasitic effects of these compounds can be confidently attributed to the inhibition of CpIMPDH. A99 is ≥17-fold selective and the remaining compounds range in selectivity from 0. 9–14-fold (Figure 5). These compounds have similar effects on both wild-type and T. gondii-ΔHXGPRT parasites (Figure 5), indicating that the low selectivity derives from off-target effects unrelated to TgIMPDH. Surprisingly, initially we did not observe a significant correlation between the potency of a compound in the enzyme assay and inhibition of T. gondii-CpIMPDH proliferation (Figure 7A). We wondered if some compounds might be binding nonspecifically to other proteins. To test this hypothesis, CpIMPDH inhibition was also evaluated in the presence of BSA [22]. A strong positive correlation is observed between inhibition of T. gondii-CpIMPDH proliferation and potency of enzyme inhibition in the presence of BSA (Figure 7B; r = 0. 94, p<0. 0001). Selectivity in the T. gondii model also correlates well with the potency of enzyme inhibition in the presence of BSA (Figure 7C; r = −0. 92, p<0. 0001). These observations indicate that the IC50 value in the presence of BSA is a useful proxy for antiparasitic activity modelled by T. gondii-CpIMPDH proliferation. Host cell growth was also assayed to assess the contribution of host cell effects to antiparasitic activity (Figures 6C and S6B). In general, strong host cell effects are observed in compounds that display little selectivity in the T. gondii model (Figures 5 & S5). With few exceptions, compounds that inhibited the proliferation of wild-type T. gondii with EC50≤10 µM also inhibited the proliferation of host cells. Compounds A82, A90 and A105 have values of EC50≤10 µM for all three Toxoplasma strains, and do not inhibit host cell growth, suggesting that their antiparasitic activities do not result from the inhibition of CpIMPDH or TgIMPDH. Instead, these compounds may act on other T. gondii targets not present in the host cell. Conversely, A100, A102, and A103 have EC50s of ≥20 µM against wild-type T. gondii yet inhibit HCT-8 cell growth significantly at 12. 5 µM and 25 µM (Figure 5). The high-content imaging assay was used to evaluate the anti-cryptosporidial activity of the 1,2, 3-triazole CpIMPDH inhibitors at 12. 5 µM and 25 µM (Figure 6B). All compounds inhibited C. parvum growth by at least 48% at a concentration of 25 µM (Figure 6B) and thus had equal or markedly improved anticryptosporidial efficacy when compared to parent compound A [20]. Unlike paromomycin, a significant reduction in parasite area was not detected (data not shown). The average area of the host cell nucleus was also recorded as a potential indicator of host cell cytotoxicity and likewise no significant change in host cell nuclei size was detected (data not shown). Encouragingly there was a negative trend between anticryptosporidial activity and host cell growth inhibition (data not shown), indicating that improvements in anticryptosporidial activity are not coincident with secondary effects on the host cell. To provide quantitative data to the SAR pipeline, the values of EC50 were determined for seven compounds. A82, A90, A92, A98 and A105 had EC50 values between 3 µM and 13 µM (Figure 5). Compounds A103 and A110 were found to be potent inhibitors of C. parvum growth with EC50 values of <0. 8 µM (Figure 8A & B). As shown above, A103 and A110 also have negligible effects on host cell growth and exhibit good selectivity in the T. gondii model. Therefore, A103 and A110 have improved specificity and efficacy, and are promising candidates for advancement into mouse models of infection. While not every compound that showed activity against the T. gondii-CpIMPDH parasite had strong anticryptosporidial activity, none of the compounds showing poor activity in the T. gondii-CpIMPDH model display significant anticryptosporidial activity. The T. gondii assay also immediately flagged compounds with poor permeability or off-target effects. We conclude that the T. gondii-CpIMPDH model provides valuable information regarding antiparasitic activity and is a fast and highly informative filter for compound progression through medicinal chemistry optimization. Despite the tremendous public health impact of cryptosporidiosis, efforts to develop new and more effective treatments for this disease have been languishing. There are a number of reasons for this, but lack of suitable tissue culture and animal models to assess drug candidates is currently the most prominent roadblock. To overcome this challenge, we have developed a facile screening pipeline to evaluate the antiparasitic activity of CpIMPDH inhibitors. The backbone of this pipeline is provided by a T. gondii model parasite that mirrors Cryptosporidium purine nucleotide pathways and depends on CpIMPDH. The T. gondii model reliably eliminates compounds from further consideration and provides a useful filter to identify off-target activities. However, efficacy in the T. gondii model does not always guarantee anti-cryptosporidial activity. This disparity likely arises from differences in the biology of the two parasites. T. gondii and C. parvum infect different tissues, and occupy different intracellular compartments. The parasitophorous membrane of T. gondii is in direct contact with the host cell cytoplasm [53]. In contrast, C. parvum remains beneath the apical membrane of the host cell and is considered ‘extracytoplasmic’ due to the presence of a parasite induced host cell actin patch along with other peculiar and still largely uncharacterized structures, including the feeder organelle and a dense band visible in electron micrographs [54], [55]. These structures separate the parasite' s parasitophorous vacuole from the host cell cytoplasm [56] and have been hypothesized to be involved in drug and nutrient uptake [57]. Furthermore, the two parasites, and their respective host cells, have different repertoires of drug efflux transporters [58], which may also account for the differences in inhibitor sensitivity. While the T. gondii assay does not fully negate the necessity of testing in Cryptosporidium directly, it has proven indispensible to winnowing candidate compounds to a number amenable to this more challenging model. We have used the pipeline to identify two promising candidates for anticryptosporidial chemotherapy: A103 and A110. These compounds are >100× more potent than paromomycin, the current standard for anticryptosporidial activity.
Persistent diarrhea is a leading cause of illness and death among impoverished children, and a growing share of this disease burden can be attributed to the parasite Cryptosporidium. There are no vaccines to prevent Cryptosporidium infection, and the treatment options are limited and unreliable. Critically, no effective treatment exists for children or adults suffering from AIDS. Cryptosporidium presents many technical obstacles for drug discovery; perhaps the most important roadblock is the difficulty of monitoring drug action. Here we have developed a set of methods to accelerate the drug discovery process for cryptosporidiosis. We exploit the opportunities for experimental manipulation in the related parasite Toxoplasma to genetically engineer a Cryptosporidium model. This new model parasite mirrors the metabolism of Cryptosporidium for a particularly promising drug target that supplies the building blocks for DNA and RNA. Drug effectiveness can be assayed through simple fluorescence measurements for many candidates. Using this assay as an initial filter, and adapting other assays to a high throughput format, we identify several novel chemical compounds that exhibit markedly improved anti-cryptosporidial activity and excellent selectivity.
infectious diseases/protozoal infections
infectious diseases/neglected tropical diseases
biochemistry/drug discovery
infectious diseases/gastrointestinal infections
A Screening Pipeline for Antiparasitic Agents Targeting Cryptosporidium Inosine Monophosphate Dehydrogenase