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Logo of nihpaAbout Author manuscriptsSubmit a manuscriptHHS Public Access; Author Manuscript; Accepted for publication in peer reviewed journal;
Nat Med. Author manuscript; available in PMC 2012 December 1.
Published in final edited form as:
PMCID: PMC3411919

A high throughput drug screen for Entamoeba histolytica identifies a new lead and target

Entamoeba histolytica, a protozoan intestinal parasite, is the causative agent of human amebiasis. Amebiasis is the fourth leading cause of death and the third leading cause of morbidity due to protozoan infections worldwide1, resulting in ~70,000 deaths annually. E. histolytica has been listed by the NIH as a category B priority biodefense pathogen in the United States. Treatment relies on metronidazole2, which has adverse effects3 and potential resistance is an increasing concern4,5. To facilitate drug screening for this anaerobic protozoan, an automated, high-throughput screen (HTS) was developed and validated. Screening identified an FDA-approved drug, auranofin, used therapeutically for rheumatoid arthritis, as active against E. histolytica in culture (EC50 0.5 µM). Auranofin was 10-times more potent against E. histolytica than metronidazole. Transcriptional profiling and direct assays indicated that auranofin likely targets the E. histolytica thioredoxin reductase (EC50 0.4 µM), preventing the reduction of thioredoxin and enhancing sensitivity of trophozoites to reactive oxygen-mediated killing. In animal models of amebic colitis and liver abscess oral auranofin significantly reduced the number of parasites, the detrimental host inflammatory response, and hepatic damage. This new use of auranofin represents a promising therapy for amebiasis, and has been granted Orphan-Drug Status from the USFDA.

Screening large chemical libraries to identify amebicidals has been hindered by the throughput of traditional assays, which were labor intensive, relying on microscopic visualization6, radioisotopes7, and/or extensive staining methods8. We have developed and employed an automated HTS that is suitable for rapid and more efficient screening of large, diverse inhibitor libraries for activity against E. histolytica. The challenges for developing the HTS platform for E. histolytica included that it is an anaerobe and that no rapid readout assay is available. These issues have been solved by the use of GasPakTM EZ Anaerobe Gas Generating Pouch Systems (VWR) and CellTiter-Glo Luminescent Cell Viability Assay (Promega). The GasPak was not needed during robotic transfers, making this assay fully compatible with workstation-based automation. The assay development was performed with exponentially growing E. histolytica trophozoites with 50,000 parasites mL−1 in 96-well8 or 15,000 mL−1 in 384-well microtiter plates. Anaerobic conditions were maintained using GasPak during growth. As ATP is an essential cofactor for biogenesis in E. histolytica, we used the luciferase-based assay to validate the correlation between the number of viable trophozoites and their ATP levels. The relationship between numbers of parasites seeded into 96- and 384-well plates and relative luminescence from CellTiter-Glo of parasites showed a linear correlation (R2 = 0.86 and R2 = 0.9) (Fig. 1a,b). Trophozoites readily tolerated up to 0.5% DMSO with no effect on growth rate. In our system, the EC50 value for metronidazole, defined as that concentration of compound necessary to reduce the culture density to 50% of that of a DMSO-treated culture, was 5 µM. This HTS assay was used to evaluate the amebicidal activity of chemicals to identify potential drug candidates and was performed with 50,000 parasites mL−1 in 96-well microtiter plate at a single concentration of 5 µM.

Figure 1
Assay development for HTS and scatter plot of percentage inhibition of each well from plates of compound library. (a) Correlation between the number of viable E. histolytica trophozoites and ATP-bioluminescence in 96-well microtiter plate. (b) Correlation ...

The screen was performed with a 910-member Iconix library, consisting of both FDA-approved and unapproved bioactive compounds. The use of drugs already approved for human use opens the possibility to rapidly and cost-effectively reprofile or repurpose9 drugs to treat amebiasis. This offers shortened development timelines and decreased risk with compounds having already passed regulatory clinical trials with full toxicological and pharmacokinetic profiles9.

Eleven compounds were identified as “active,” causing statistically significant growth inhibition (> 50%; Fig. 1c and Table 1). The assay showed excellent discrimination between active and inactive compounds with a Z′ factor of 0.96±0.13 in the screening experiment using 12 different plates. Among 11 compounds, auranofin demonstrated the highest amebicidal activity with an EC50 of 0.5 µM, 10-fold better than the current drug of choice, metronidazole. Repurchased auranofin and three auranofin analogs also inhibited growth of E. histolytica trophozoites (Supplementary Table 1). Two purine analogs, cladribine and fludarabine, showed 79% and 77% inhibition at 5 µM, respectively, but are not promising for further development because of reported adverse effects on patients. Trifluoperazine, a compound with known amebicidal activity10 was also identified as a primary hit, confirming the sensitivity of our whole cell HTS assay format.

Table 1
Hits obtained after screening the Iconix library

Auranofin is an FDA-approved oral, gold-containing drug that has been in clinical use to treat rheumatoid arthritis (RA) for 25 years and is sold as RidauraTM (Prometheus Laboratories). The published pharmacokinetic data of auranofin comes from studies in RA patients following long-term therapy. Auranofin is rapidly metabolized so no intact drug can be detected, but gold levels have been measured. Following an oral dose, 25% of auranofin is absorbed, 60% is plasma protein bound, and 85% excreted in feces11. Steady-state mean blood gold levels are 0.68±0.45 µg mL−1 (package insert) or approximately 3.5 µM, more than seven times the EC50 for E. histolytica. Auranofin was approved for the long-term treatment of unresponsive RA with courses for a minimum of 6 months at doses of 3 mg once or twice a day. The complications listed in the package insert for long-term (> 1 yr) auranofin therapy include dermatologic: rash (26%); gastrointestinal: loose stools (42%), abdominal pain (14%), nausea (10%); hematologic: anemia, leucopenia, thrombocytopenia in up to 3%; hepatic: elevated liver enzymes (2%); mucous membranes: stomatitis (13%); renal: proteinuria (1%). The likelihood of gold toxicity is extremely small in short-term (7–10 d) therapy for amebiasis.

Recently, auranofin has been shown to rapidly kill juvenile and adult Schistosoma mansoni in culture at physiological concentrations (5 µM)12, as well as bloodstream and procyclic stages of Trypanosoma brucei13. Concentrations as low as 2.5 µM also killed larval worms of Echinococcus granulosus14. Auranofin also strongly inhibited the growth of malarial parasite Plasmodium falciparum in vitro15 and killed the promastigote stage of Leishmania infantum at micromolar concentration16.

Despite 25 years of clinical use, the mechanism of action of auranofin is poorly understood. To identify the basis of auranofin activity versus E. histolytica, a transcriptional profiling study was undertaken using E. histolytica oligonucleotide microarrays17. Incubation of E. histolytica with auranofin for only 3 h at 1 µM concentration identified auranofin-induced downregulation of critical genes involved in mitosis (Rae118) and nucleotide metabolism (nucleoside diphosphate kinase19), while signal transduction genes encoding ADP-ribosylation factor and Ras1p were upregulated20 (Supplementary Table 2). However, these transcripts are also induced by other forms of cellular stress. Furthermore, there was a marked upregulation of the gene encoding a protein similar to arsenite-inducible RNA-associated protein (AIRAP) (Supplementary Table 2). The differential expressions of these transcripts were validated by quantitative real-time PCR (qRT-PCR) (Supplementary Fig. 1 and Supplementary Table 3).

AIRAP is unique among known arsenite-induced genes in that expression is not upregulated in response to other oxidants and is only modestly induced by exposure to other metals, such as zinc21. We have shown that the transcript for a gene similar to AIRAP in E. histolytica was highly upregulated by treatment with low concentrations of auranofin, thereby identifying a novel gene in E. histolytica selectively inducible by auranofin exposure. It is noteworthy that both arsenite and auranofin are reported to be inhibitors of thioredoxin reductase (TrxR)22,23 and metabolic inhibitors of selenium metabolism24. This led us to hypothesize that E. histolytica TrxR likely is the target for auranofin. Because E. histolytica resides in either aerobic (liver) or anaerobic environments (colon) in their mammalian hosts, they must have means to minimize damage caused by reactive oxygen species produced by the host immune assault. In most organisms there are two largely independent systems to detoxify reactive oxygen species, one based on glutathione and the other based on thioredoxin. Each of these systems has a dedicated NADPH-dependent flavoenzyme, glutathione reductase and TrxR, to maintain the reduced state of glutathione or thioredoxin, respectively257. However, E. histolytica lacks both glutathione reductase activity and glutathione synthetic enzymes28; its TrxR is involved in prevention, intervention and repair of damage caused by oxidative stress29.

There is a single TrxR-encoding gene in the E. histolytica genome (23.m00296), which belongs to the low molecular weight TrxR family30, and is similar to bacterial and yeast enzymes, including the TrxR from Escherichia coli (Supplementary Fig. 2). In contrast, most higher eukaryotes have a high molecular weight TrxR which is typically a selenocysteine protein; this enzyme in S. mansoni, known as TGR, has both Se and an appended glutaredoxin domain23 (Supplementary Fig. 3). We hypothesized that EhTrxR would not contain selenium and that auranofin would bind to the active site cysteines. Active, His-tagged EhTrxR was readily purified from solubilized E. coli by nickel-affinity chromatography, with properties similar to those previously reported for EhTrxR29.

The activities of auranofin and its two most active analogs were examined for inhibition of recombinant EhTrxR. Low µM concentrations of auranofin and analog 39 and nM concentrations of analog 7 were inhibitory (Fig. 2a–c). The assays were non-linear for the first 50 s, unlike control reactions without auranofin; inhibition increased with time until a linear, inhibited rate was established after 50 s of reaction (Fig. 2a, inset). Examination of the rates after 50 s indicated that 0.4 µM auranofin caused 50% inhibition. Preincubation of the inhibitor with reduced EhTrxR did not remove the lag phase in inhibition as seen by the nonlinearity of the data acquired up to 50 s (not shown).

Figure 2
Inhibition of EhTrxR by auranofin and its analogs. The indicated concentrations of auranofin and analogs were incubated with 45 nM (a,b) or 20 nM EhTrxR (c), 20 µM E. coli Trx1 and 200 µM DTNB for 3 min before addition of NADPH to initiate ...

Because TrxR is critical for protecting amebic trophozoites from oxidant attack, we compared the susceptibility of trophozoites with and without auranofin treatment to reactive oxygen species using H2O2. Following incubation of trophozoites with 2 µM auranofin for 18 h, the remaining viable trophozoites (~50%) were significantly more sensitive to killing by 300 µM H2O2 than control trophozoites in media alone (P < 0.002) (Fig. 2d). Killing by auranofin (2 µM) and H2O2 was reversed by the presence of 2 mg mL−1 of cysteine (Fig. 2d). Cysteine is the major reductant in the trophozoite31, and its apparent protective effect may be through direct reduction of thioredoxin or inhibition of auranofin binding to cysteine residues in TrxR. The presence of reactive oxygen species due to 2 µM auranofin treatment could be detected with fluorescence generated by the oxidation of dichlorodihydrofluorescein32 (Fig. 2e). However, the same concentration of metronidazole, although producing stress, did not increase intracellular reactive oxygen species (Supplementary Fig. 4). Moreover, increased oxidized thioredoxin was observed in auranofin-treated trophozoites, both in vitro and in vivo, indicating that TrxR likely is a target for auranofin (Fig. 2f).

Recently, Angelucci et al23, solved the crystal structure of S. mansoni TGR that had been incubated with auranofin before crystallization. The structure revealed gold [Au(I)] rather than auranofin as an adduct between pairs of cysteines (Cys-gold-Cys) in two different sites and also bound to the proposed NADPH binding site of the reductase in a third location. The C-terminus of TGR containing a selenocysteine residue was not observed in the structure and may have bound a fourth gold atom. Angelucci et al23 proposed that the selenocysteine at the penultimate position of TGR accelerated the release of gold from auranofin to form the inactivated enzymes; benzeneselenol added to a C-terminally truncated TGR or to glutathione reductase increased the rate of inactivation by auranofin. The crystal structure of reduced L. infantum trypanothione reductase in complex with NADPH and auranofin also demonstrated that gold binds to two active cysteine residues of trypanothione reductase16.

EhTrxR is of very similar size and domain topology as E. coli TrxR, a well-studied enzyme33. Both proteins have an active site dithiol/disulfide center (CATC for EcTrxR, CAIC for EhTrxR) plus either two or four additional Cys residues, respectively (Supplementary Fig. 2). By analogy with the S. mansoni TGR, addition of auranofin could cause gold atoms to bind to the NADPH-binding site of EhTrxR, to the active site thiols, to the four Cys residues near the C-terminus of the enzyme, or to some combination of these sites.

Because of auranofin’s in vitro activity against E. histolytica trophozoites and oral availability, we tested its efficacy in two animal models of amebiasis. We adapted a murine amebic colitis model, in which trophozoites invade and colonize mouse cecal tissue following surgical inoculation34,35. Amebic trophozoites were co-cultured with cecal bacteria and surgically inoculated into the cecum of C3H/HeJ mice. Auranofin or metronidazole were delivered by gavage 24 h after infection at a concentration of 1 mg kg−1 d−1 for 7 d36. Both the parasite burden and the inflammatory response as measured by myeloperoxidase were significantly reduced by auranofin (P = 0.037 and 0.0021) (Fig. 3a,b) but not by metronidazole (Fig. 3c,d). Auranofin (Fig. 3e) was more effective than an equivalent dose of metronidazole (Fig. 3f) in a hamster model of amebic liver abscess where treatment started 4 d after infection. A single oral dose of 3 mg kg−1 d−1 of auranofin for 7 d significantly decreased hepatic damage in hamsters (P = 0.002) (Fig. 3e). These findings suggest that auranofin may be an entirely new class of drug to treat amebiasis and potentially other parasitic infections. Based on these results, the USFDA has approved an Orphan-Drug designation of auranofin for treatment of amebiasis.

Figure 3
Effect of auranofin or metronidazole on animal models of amebic colitis and liver abscesses. The treatment of mice with cecal amebiasis with auranofin (a,b) or metronidazole (c,d) is presented as the percentage of trophozoites gm−1 of tissue or ...

In summary, we have shown that it is feasible to screen large numbers of compounds in an HTS-format versus E. histolytica and robust and reproducible results can be generated from this HTS. The discovery of the amebicidal activity of the FDA-approved drug auranofin and its recent orphan-drug designation offer a promising drug repositioning opportunity for the treatment of amebiasis.


E. histolytica cultures

Axenic E. histolytica (HM1:IMSS) trophozoites were maintained in TYI-S-33 medium38 and counted using a particle counter (Beckman Coulter).

Compound libraries

A library of 910 bioactive compounds was donated by Iconix Biosciences.

HTS cell viability assay

Compounds were diluted using a Biomek FXp Laboratory Automation Workstation (Beckman Coulter) and the Matrix WellMate bulk dispenser (Thermo Fisher Scientific) to yield 125 µM compound in 12.5% DMSO. Finally, FXp transferred 4 µL of diluted compound to the 96-well screen plates, followed by addition of 96 µL (5,000 parasites) of E. histolytica trophozoites in TYI-S-33 complete medium to the 96-well plates, by the WellMate. Final concentrations of test compound and DMSO per well were 5 µM and 0.5%, respectively.

Negative controls in the screen plates contained 0.5% DMSO and positive controls contained 30 µM metronidazole (Sigma). Assay plates were incubated for 48 h at 37 °C in the GasPak to maintain an anaerobic condition throughout the incubation period. At the end of incubation, the assay plates were equilibrated to room temp. for 30 min, 50 µL of CellTiter-Glo were added in each well of the 96-well plates, using the WellMate. The plates were then placed on an orbital shaker at RT for 10 min to induce cell lysis. After lysis, the plates were again equilibrated at RT for 10 min to stabilize the luminescent signal. The resulting ATP-bioluminescence of the trophozoites was measured at RT using an Analyst HT plate reader (Molecular Devices).

Secondary screen for potency determination

For confirmatory screens of trophozoites, hits from the primary screen were picked from 5 mM stocks in 100% DMSO using the Biomek FXp. For 8-point EC50 determination experiments, we diluted 2.5 µL of stock compounds with 17.5 µL sterile water to yield 625 µM working concentration of library compounds. A three-fold serial dilution was then performed yielding a concentration range 0.25–625 µM. From this dilution plate, 4 µL were transferred into the 96-well screen plates followed by addition of 96 µL of trophozoites (5,000 parasites) to yield a final 8-point concentration range spanning 0.01–25 µM in final 0.5% DMSO. The assays were performed in triplicate using CellTiter-Glo. Visualization and statistical analysis of secondary screening were performed using GraphPad Prism software 4.0.

HTS data analysis and statistics

The raw data file from the Analyst HT plate reader was uploaded using Pipeline Pilot 4.5.2 into Small Molecule Discovery Center’s database (MySQL). The results are posted ( with tables, Z′, heat maps, scatter plots, and percent inhibition relative to maximum and minimum reference signal controls. Percent inhibition relative to maximum and minimum reference signal controls was calculated using the formula:

  • % Inhibition = [(mean of Maximum Signal Reference Control − Experimental Value)/(mean of Maximum Signal Reference Control − mean of Minimum Signal Reference Control)] × 100

The cutoff was selected to determine actives from the primary screen, which was at least 50% inhibition and 3 standard deviations above the mean of the population of compounds tested.

E. histolytica microarray analysis

We used E. histolytica oligonucleotide arrays for characterizing transcriptional effects of auranofin. These microarrays were composed of 6209, 70 mer oligonucleotides and encompassed approximately 90% of the unique genes found in the E. histolytica genome dataset as of February 2004. Oligonucleotides were printed in triplicate on slides by the Washington University School of Medicine Microarray Core Facility17. We isolated total RNA from 3 h 0.5% DMSO-treated 2 × 106 E. histolytica HM1:IMSS and 3 h 1 µM auranofin-treated 2 × 106 HM1 using TRIZOL (Invitrogen). Total RNA was amplified with the Amino Allyl MessageAmp™ II aRNA Amplification Kit (Ambion) following the manufacturer’s protocol. The monofunctional NHS-ester Cy3 and Cy5 dyes (GE Healthcare Life Sciences) were coupled with 10 µg amplified RNA. The two aRNA pools to be compared were mixed and applied to E. histolytica microarray. Four samples (two from DMSO-treated and two from auranofin-treated) were competitively hybridized on two individual chips. The hybridization was performed at 63 °C for 16 h in a humidified slide chamber containing the labeled probe, 3X SSC, and 0.2% SDS. After hybridization, the hybridization chamber was removed from the 63 °C water bath, washed with 0.6X SSC, 0.03% SDS, and then 0.06X SSC. Microarrays were scanned using a GenePix Pro Axon 4000B scanner, data were analyzed (Acuity software, Molecular Devices) and deposited in the public database ArrayExpress ( under the accession number E-MEXP-3494.


We isolated total RNA from control and auranofin-treated trophozoites (above). After reverse transcription, we performed qRT-PCR using SYBR Green I Master (Roche Applied Science) and the PCR product was monitored (Mx3005PTM QPCR System with MxProTM QPCR software, Stratagene). Primer sequences are in Supplementary Table 3.

Purification of recombinant E. histolytica TrxR

The EhTrxR coding sequence was amplified29 from genomic DNA35, cloned into pET22b (Novagen) and transformed into BL21 Codon Plus cells (Stratagene). Protein expression was induced (1 mM IPTG, 2 h, 37 °C), the pellet lysed in B-PER (Thermo Scientific), and soluble EhTrxR (1% Triton X-100, 10 mM imidazole) purified by NiNTA affinity chromatography (Qiagen).

E. histolytica TrxR assay

The thionitrobenzoate-coupled assay for TrxR activity was modified from Mulrooney39. Briefly, 600 µL total of 50 mM potassium phosphate, pH 7.0, 1 mM EDTA contained 20 µM E. coli Trx1, 200 µM 5,5′-dithiobis(2-nitrobenzoic acid) (DTNB) and 20 or 45 nM EhTrxR at 25 °C. The reaction was started by addition of 100 µM NADPH and monitored by 412 nm absorbance, which increases with reaction due to DTNB reduction. With these concentrations of DTNB and EhTrxR, in the absence of EcTrxA there was a negligible increase in 412 nm absorbance. When present, the indicated concentration of auranofin (predissolved in ethanol) was added 3 minutes before the NADPH (to a maximum added volume, at 3.6 µL, of 0.6% of the total). The initial rate and the rate after 50 s were calculated from the increase in 412 nm absorbance, using an extinction coefficient for nitrothiobenzoate anion of 13,600 M−1 cm−1 (with 2 molecules of nitrothiobenzoate generated per NADPH oxidized) to convert the absorbance change to rates in nmol NADPH min−1.

Auranofin effect on trophozoites

To determine the effect of auranofin on oxidant stress, we pre-incubated trophozoites (5 × 105 in TYI-S-33) at 37 °C with auranofin (2 µM, 18 h), ethanol, or TYI-S-33 containing 2 mg mL−1 of cysteine (Sigma). Trophozoites were then counted, viability assessed by trypan blue exclusion, and resuspended in TYI-S-33 with 300 µM H2O2. Aliquots were removed in triplicate every 30 min for 2 h and % survival determined with the CellTiter-Glo with statistical analysis by Student’s t test.

We determined intracellular oxidant levels incubating control (ethanol), ethanol + H2O2−, auranofin-, and auranofin + H2O2-treated trophozoites with 0.2 mM 2′,7′-dichlorodihydro-fluorescein diacetate (Sigma) for 45 min32, washing, fixing with 4% paraformaldehyde, resuspending in ProLong Gold mounting media with nuclear stain (DAPI) and examining by a Nikon E800 fluorescence microscope.

The redox state of thioredoxin in amebic trophozoites was determined by protein electrophoretic mobility shift assay37. HM-1 trophozoites were incubated 18 h with auranofin (2 µM) or media alone. In vivo trophozoites were obtained by flushing infected mice cecum after treatment for 48 h with auranofin at 1 mg kg−1 or the ethanol vehicle alone. Trophozoites were washed in PBS, pH 7.4, lysed in 100 mM Tris, 8 M urea, 1 mM EDTA and 30 mM iodoacetic acid, pH 7.2 for 37 °C for 15 min., excess IAA removed by precipitation in cold acetone/1 N HCl (98:2, v/v) and washed in acetone/1 N HCl, water (98:2:10). The disulfides were subsequently reduced in the urea buffer containing 3.5 mM DTT for 30 min at 37 °C, and the new thiols amidomethylated with 10 mM iodoacetamide. Markers were prepared by incubating cultured trophozoites in urea buffer with 3.5 mM DTT for 30 min at 37 °C, then equal aliquots alkylated with 30 mM iodoacetic acid (reduced marker) or 10 mM iodoacetamide (oxidized) marker for 30 min at 37 °C37. Samples were electrophoresed by native urea-PAGE on 9% gels, transferred to nitrocellulose and the bands detected with rabbit EhTrx-specific antibody29 (1:200) and goat anti-rabbit horseradish peroxidase (Invitrogen, 1:10,000) by enhanced chemiluminescence (SuperSignal, West Pico, Fisher Scientific).

In vivo efficacy of auranofin

We injected cecal-passed trophozoites into the externalized cecum of six-week-old C3H/HeJ male mice34 (The Jackson Laboratory) and treated orally 24 h after infection with 1 mg kg−1 d−1 auranofin (Enzo Life Sciences) or metronidazole for 7 d. The mice were then sacrificed, the cecum removed for histopathology, quantification of trophozoites by real-time PCR, and myeloperoxidase (MPO) activity40. Mouse studies were approved by the UCSD Institutional Animal Care Committee.

We injected trophozoites (250,000 in 0.2 mL TYI-S-33) intraportally in hamsters to induce liver abscesses. The hamsters were treated 4 d after infection orally with 3 mg kg−1 of auranofin, metronidazole, or PBS daily for 7 d. The hamsters were sacrificed and the livers and abscesses were dissected and weighed. Hamster studies were approved by the CINVESTAV-IPN Internal Committee for the Care and Use of the Laboratory Animals.

Supplementary Material


This work was supported by the Sandler Foundation and NIAID 5U01AI077822-02; support from R01 GM050389 is also acknowledged. E. histolytica microarray slides were kindly provided by S. L. Stanley Jr. of Stony Brook University, New York, and the E. histolytica thioredoxin-specific antibody a kind gift from S. Adrian-Guerrero of the Universidad Nacional del Litoral, Santa Fe, Argentina. We thank, G. Hwang and C. Le for their help with the animal surgery, and K. Ang and J. Gut for sharing their expertise.



A.D. and J.H.M. designed the HTS screening studies, arrays, which A.D. performed. D.P. and L.B.P. performed the enzymatic assays. R.M.A. performed the oxidant studies. C.H., E.R.C., K.H., G.G.-R., E.O. and M.B.M. did the in vivo studies. K.H. purified rEhTrxR. S.C. and M.R.A. provided compound libraries and edited the manuscript. S.S.G. and A.M.B. synthesized auranofin analogs. S.L.R. designed the EhTrxR and oxidant studies. A.D., L.B.P., J.H.M. and S.L.R. wrote the manuscript.


The authors declare that they have no competing financial interest.


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