In response to the current global health emergency posed by the Zika virus (ZIKV) outbreak and its link to microcephaly and other neurological conditions, we performed a drug repurposing screen of 6,000 compounds that included approved drugs, clinical trial drug candidates and pharmacologically active compounds; we identified compounds that either inhibit ZIKV infection or suppress infection-induced caspase-3 activity in different neural cells. A pan-caspase inhibitor, emricasan, inhibited ZIKV-induced increases in caspase-3 activity and protected human cortical neural progenitors in both monolayer and three-dimensional organoid cultures. Ten structurally unrelated inhibitors of cyclin-dependent kinases inhibited ZIKV replication. Niclosamide, a category B anthelmintic drug approved by the US Food and Drug Administration, also inhibited ZIKV replication. Finally, combination treatments using one compound from each category (neuroprotective and antiviral) further increased protection of human neural progenitors and astrocytes from ZIKV-induced cell death. Our results demonstrate the efficacy of this screening strategy and identify lead compounds for anti-ZIKV drug development.


ZIKV, a mosquito-borne flavivirus, has spread across the Western Hemisphere in the past year. First isolated in 1947 from a sentinel rhesus macaque in the Ziika Forest region of Uganda1, ZIKV remained in relative obscurity for many years until outbreaks occurred in the Pacific islands and then in the Americas in the past decade. A large outbreak started in Brazil in late 2014, and it is a growing public health concern2. Active transmission has been reported in approximately 60 countries and territories globally. Most human infections are transmitted by mosquitos; however, ZIKV can also spread directly through sexual contact3,4,5,6 and vertically from mother to fetus7,8,9. About 20% of ZIKV-infected individuals develop symptoms, which mostly resemble those caused by other arboviruses, such as dengue viruses or chikungunya virus. Unlike these viruses, however, ZIKV causes congenital defects, including microcephaly10,11, and is associated with Guillain–Barré syndrome, meningoencephalitis and myelitis in infected adults8,11,12,13,14.

Since the recent declaration by the World Health Organization (WHO) that ZIKV is a global health concern, rapid progress has been made to understand its pathogenesis and to develop human in vitro models and animal in vivo models15,16,17,18,19,20,21,22,23. Following clinical observations of ZIKV in fetal brains obtained from infected women9,10, we reported that ZIKV efficiently targets human neural progenitor cells (hNPCs) and attenuates their growth15. This finding provides a potential mechanism for ZIKV-induced microcephaly as hNPCs drive the development of the cortex in the human brain. Furthermore, we and others have shown that ZIKV infection of brain organoids, which are used as three-dimensional (3D) cellular models of early human brain development, leads to reduced thickness of hNPC and neuronal layers, and an overall reduction in organoid size16,17,20,24, observations that are again consistent with features of microcephaly. These results have also been recapitulated in mouse models20,21,23. Despite these advancements in understanding how ZIKV causes developmental abnormalities and in preclinical studies that are underway to develop vaccines25,26, there is currently no drug approved to treat or prevent ZIKV infection.

Drug repurposing screens have recently emerged as an alternative approach to accelerate drug development27,28. Following a repurposing phenotypic screen, new indications for existing drugs may be rapidly identified, and clinical trials can be carried out quickly, which is especially critical for rapidly spreading infectious diseases. For example, recent drug repurposing screens have led to discoveries of potential new candidate therapies for Ebola virus disease29,30, giardiasis31, Entamoeba histolytica infection32, malaria gametocytes33, Exserohilum rostratum infection34, hepatitis C virus (HCV) infection35 and, very recently, ZIKV infection36. On the basis of our previous finding that ZIKV infection of hNPCs results in an increase in caspase-3 activation, followed by cell death15, we designed a compound-screening approach using caspase-3 activity as the primary screening assay, with a secondary cell viability assay for confirmation (Supplementary Fig. 1a). We identified two classes of effective compounds that are capable of protecting neural cells from ZIKV-induced cell death, one consisting of compounds that are antiviral in nature and the other of compounds that are neuroprotective in nature.


Development of high-throughput compound-screening approaches

We first quantified caspase-3 activity and cell viability in hNPCs and astrocytes that were derived from human induced pluripotent stem cells (iPSCs), as well as in glioblastoma SNB-19 cells, after ZIKV infection in a 1,536-well plate format (Supplementary Tables 1 and 2). The prototypic ZIKV strain, MR766, was used in the primary screen because it produced the strongest cell death signal in cell culture experiments. The signal-to-basal (S/B) ratios and the coefficients of variation (CV) obtained in the caspase-3 activity assay after a 6-h ZIKV exposure were 2.1-fold and 7.0% for hNPCs, 7.0-fold and 5.9% for SNB-19 cells and 11.0-fold and 9.1% for astrocytes (Supplementary Fig. 1b). The Z′ factors, which are a measure of statistical effect size and an index for assay quality control37, for hNPCs, SNB-19 and astrocytes were 0.20, 0.68 and 0.72, respectively. Because a Z′ factor >0.5 indicates a robust screening assay37, the caspase assay using SNB-19 cells or astrocytes is suitable for high-throughput screening.

To measure cell viability, we performed an ATP-content assay following ZIKV infection for 3 d (Supplementary Table 2). Cell viability was reduced by 39%, 82% and 69% in hNPCs, SNB-19 cells and human astrocytes, respectively (Supplementary Fig. 1c). The Z′ factors in these three cell types were 0.06, 0.37 and 0.32, respectively. These results indicated that measuring caspase-3 activity is a better assay for high-throughput compound screening than the cell-viability assay.

High-throughput screen of compound collections

We carried out a screening campaign, using the caspase-3 activity assay and SNB-19 cells, with the Library of Pharmacologically Active Compounds (LOPAC, 1,280 compounds), the National Center for Advancing Translational Sciences (NCATS) Pharmaceutical Collection of approved drugs (2,816 compounds) and a collection of clinical candidate compounds (2,000 compounds). Primary hits included a total of 116 compounds that suppressed ZIKV-induced caspase-3 activity in SNB-19 cells. We also carried out an independent primary screen in hNPCs using the same libraries. This second screen resulted in 173 primary hits that included all 116 compounds from the initial caspase-3 screen in SNB-19 cells. All of the results from the primary screen with the approved drug collections, and hit confirmation, were deposited into the open-access PubChem database (https://pubchem.ncbi.nlm.nih.gov/).

Next, the activity of these primary hits from the caspase-3 activity assay was re-evaluated in ZIKV-infected SNB-19 cells, hNPCs and astrocytes, and, notably, was performed in parallel with the compound cytotoxicity assay (Supplementary Fig. 1d,e and Supplementary Table 3). Cytotoxic compounds were then eliminated from the confirmed-hit list. Consistent with the screening design, we identified compounds that reduced virally induced caspase activation and apoptosis by either directly preventing ZIKV-induced cell death or suppressing ZIKV replication (Supplementary Table 4).

Protection from ZIKV-induced cell death by emricasan

Emricasan, a pan-caspase inhibitor, was identified as the most potent anti-cell-death compound, with half-maximal inhibitory concentration (IC50) values of 0.13–0.9 μM in both caspase activity and cell viability assays for SNB-19 cells against three ZIKV strains: MR766 (1947 Ugandan strain), FSS13025 (2010 Cambodian strain) and PRVABC59 (2015 Puerto Rican strain) (Fig. 1a). It was also effective for all three cell types tested (Supplementary Fig. 1f and Supplementary Table 5). In addition, emricasan treatment reduced the number of active (cleaved) caspase-3-expressing forebrain-specific hNPCs after infection with FSS13025, in both monolayer and 3D organoid cultures (Fig. 1b,c). Emricasan treatment of ZIKV-exposed brain organoids did not seem to affect hNPC proliferation, as compared to the mock-treated organoids, when evaluated by phospho-histone3 (PH3) expression (106 ± 10%; n = 8; P = 0.7; one-way analysis of variance (ANOVA)). Notably, ZIKV antigen persisted in both 2D and 3D cultures after emricasan treatment (Fig. 1b,c). Therefore, emricasan shows neuroprotective activity for hNPCs but does not suppress ZIKV replication.

Figure 1: Emricasan suppresses cell death of ZIKV-infected human astrocytes and hNPCs in 2D monolayer cultures and in 3D brain organoids.
Figure 1

(a) Top, chemical structure of emricasan. Bottom, dose-response curves showing the effect of emricasan treatment on caspase activity (middle) and cell viability (bottom) in SNB-19 glioblastoma cells exposed to three different ZIKV strains. Values represent mean ± s.d. (n = 3 cultures). Curves represent best fits for calculating the IC50 values, and the insets in each graph report the calculated IC50 value against each strain. RLU, relative luminescence units. (b) Left, representative images of 2D monolayer cultures of forebrain-specific hNPCs immunostained for ZIKV protein (ZIKVE; green), cleaved caspase-3 (CAS3; red) and nuclei (with DAPI; gray) 72 h after ZIKV FSS-13025 exposure (with or without emricasan treatment) or mock infections (multiplicity of infection (MOI) = 0.04–0.08). Scale bar, 20 μm. Right, quantification of the percentage of CAS3+ cells, relative to the total number of DAPI-stained cells, in mock or ZIKV-infected hNPCs cultures treated with the indicated concentrations of emricasan (n = 3 cultures). Values represent mean ± s.e.m. **P < 0.01; by one-way ANOVA. (c) Left, representative images of 3D human forebrain-specific organoid cultures (28 d in vitro) immunostained for ZIKVE (green), CAS3 (red) and nuclei (with DAPI; gray), 10 d after ZIKV FSS-13025 exposure. Scale bar, 100 μm. Right, quantification of the percentage of CAS3+ cells, relative to the total number of DAPI-stained cells, in the ventricular zone (n = 6 organoids). Values represent mean ± s.e.m. ***P < 0.001; by one-way ANOVA.

Identification of antiviral compounds against ZIKV

Using expression of ZIKV protein NS1 as a read-out to screen anti-ZIKV activity, we identified two compounds from the primary hit list that substantially inhibited ZIKV infection of SNB-19 cells (Supplementary Fig. 2a). The first was niclosamide, a US Food and Drug Administration (FDA)-approved drug for treating worm infections in both humans and domestic livestock; the other was PHA-690509, an investigational compound that functions as a cyclin-dependent kinase inhibitor (CDKi). Both compounds inhibited replication of all three strains of ZIKV, as measured by NS1 expression, in a dose-dependent manner (Fig. 2a–d and Supplementary Fig. 2b,c).

Figure 2: Identification of PHA-690509 and niclosamide as antiviral compounds.
Figure 2

(a) Top, representative western blot analysis for anti-ZIKV activity after treatment of SNB-19 cells with varying concentrations of PHA-690509. Glioblastoma SNB-19 cells were treated with the indicated compound for 1 h before inoculation with ZIKV FSS-13025, PRVABC59 or MR766 (MOI = 1), and cells were harvested 24 h after infection for western blot analysis. Bottom, quantification of NS1 protein band intensities, relative to those of GAPDH (n = 3 cultures). Data were normalized to that for DMSO-treated cells. Values represent mean ± s.d. ***P < 0.001; by one-way ANOVA in comparison to DMSO-treated cells. Inset shows chemical structure of PHA-690509. (b) Top, representative western blot images of titration for anti-ZIKV activity after treatment of SNB-19 cells with emricasan. Bottom, quantification as in a (n = 3 cultures). Values represent mean ± s.d. P > 0.1; by one-way ANOVA, as compared to DMSO-treated cells. (c) Top, chemical structure of niclosamide and representative western blot images for anti-ZIKV activity after treatment of SNB-19 cells with varying concentrations of niclosamide, using the PRVABC59 strain (MOI = 1). Bottom, quantification as in a (n = 3 cultures). Values represent mean ± s.d. **P < 0.01; ***P < 0.001; by one-way ANOVA, as compared to DMSO-treated cells. (d) Summary of ELISA quantifications of secreted ZIKV NS1 protein in the medium of infected cells after treatment of cells with different doses of niclosamide (left) or PHA-690509 (right) for 24 h (n = 3 cultures). Values represent mean ± s.d. ***P < 0.001; by one-way ANOVA, as compared to the 0 μM group. (e) Summary of titration of niclosamide and PHA-690509 on ZIKV production. SNB-19 cells were treated with each indicated compound at increasing concentrations for 1 h before infection with PRVABC59 at a MOI = 0.5 (n = 3 cultures). Cell culture supernatant was collected 24 h after infection, and infectious virions were quantified for focus-forming units (FFU) using Vero cells. Data represent mean ± s.d. Curves represent best fits for calculating IC50 values, and the insets report the calculated IC50 value for each compound.

We further validated the antiviral activity of these two compounds using independent approaches. First, measurement of intracellular ZIKV RNA levels showed IC50 values of 1.72 μM and 0.37 μM for PHA-690509 and niclosamide, respectively (Supplementary Fig. 2d,e). Second, both compounds suppressed production of infectious ZIKV particles at submicromolar concentrations (Fig. 2e). To investigate the underlying cellular mechanism, we performed time-of-addition experiments in SNB-19 cells (Fig. 3a). Both compounds effectively inhibited ZIKV infection when added either 1 h before or 4 h after virus inoculation (Fig. 3b). In contrast, a monoclonal antibody to AXL, a putative ZIKV entry factor38,39, was only effective when added before inoculation (Fig. 3b). Furthermore, the reduction of ZIKV RNA by treatment with these compounds was apparent only after the entry phase (0–4 h after infection) and correlated with the replication phase (4–24 h) of the infection cycle (Supplementary Fig. 3). Taken together, these results indicate that niclosamide and PHA-690509 inhibit ZIKV infection at a post-entry stage, probably at the viral RNA replication step.

Figure 3: Inhibition of ZIKV infection by niclosamide and PHA-690509 at a post-entry step and blockade of ZIKV infection by additional treatment with CDKis.
Figure 3

(a) Schematic illustration of a time-of-addition experiment for treatment with niclosamide and PHA-690509. (b) Top, representative western blot images of SNB-19 cells after treatment with 10 μg/ml AXL-specific antibody, 2 μM niclosamide (Niclo.) or 92 μM PHA-690509 for 1 h before or 4 h after infection with PRVABC59 (MOI = 1). Bottom, quantification of NS1 protein band intensities, relative to those for GAPDH (n = 3 cultures). Data were normalized to those obtained for DMSO-treated cells. Values represent mean ± s.d. *P < 0.05; **P < 0.01; ***P < 0.001; by one-way ANOVA, as compared to DMSO-treated cells. (c) Inhibition of ZIKV infection in CDKi-treated cells. Left, representative western blot images of SNB-19 cells treated with 92 μM of the indicated compound for 1 h before infection with FSS13025 or PRVABC59 (MOI = 1). Right, quantification as in b. Values represent mean ± s.d. (n = 3 cultures; ***P < 0.01; one-way ANOVA for comparison with the DMSO treatment). (d) Effect of various CDKis on ZIKV production (as in Fig. 2e) (n = 3 cultures). All data were normalized to that for 0 μM for each compound. Data represent mean ± s.d. Curves represent best fits for calculating IC50 values (listed to the right).

Pharmacological CDKis have been shown to inhibit replication of diverse viruses in culture, including herpes viruses and HIV40,41,42,43,44,45, and depletion of CDK9 impairs influenza A viral replication46. The possibility of ZIKV inhibition by a CDKi is particularly intriguing, given our recent observation that ZIKV infection and cell cycle regulation are intimately connected15. We therefore tested 27 additional structurally distinct CDKis for inhibition of ZIKV infection (Supplementary Table 6). We identified nine effective compounds using SNB-19 cells (Fig. 3c,d and Supplementary Fig. 4a), whereas four non-CDK-kinase inhibitors showed minimal anti-ZIKV activity (Supplementary Fig. 4b). Analyses of ZIKV production showed IC50 values at submicromolar concentrations for nine of the ten CDKis tested, with seliciclib and RGB-286147 at 24 nM and 27 nM, respectively (Fig. 3d).

Using the clinical isolate from the 2015 Puerto Rico Zika outbreak, PRVABC59, we next examined the effectiveness of the identified compounds in hNPCs and astrocytes, both of which are target cells for ZIKV infection in the fetal brain9. Niclosamide and PHA-690509 treatments inhibited ZIKV infection and production in these central nervous system cells (Fig. 4a–c). ZIKV targets astrocytes in the adult mouse brain47. Analysis of ZIKV production after infection of human astrocytes showed IC50 values of 0.2 μM for both niclosamide and PHA-690509 (Fig. 4c). Quantification of astrocyte viability showed minimal toxicity for niclosamide, PHA-690509 and four CDKis at levels <3 μM (Supplementary Fig. 5a). Given the critical role of CDKs in cell cycle regulation, we examined the effect of PHA-690509 and seliciclib, the most potent CDKi for ZIKV inhibition (Fig. 3d), on hNPC proliferation. ZIKV infection led to a drastic reduction in hNPC proliferation, which was partially rescued by treatment with either compound (Supplementary Fig. 5b). Furthermore, treatment with PHA-690509 (1 μM) or seliciclib (5 μM) alone had minimal effect on hNPC proliferation in brain organoids (Supplementary Fig. 5c).

Figure 4: Niclosamide and PHA-690509 inhibit ZIKV infection in human astrocytes and forebrain-specific hNPCs.
Figure 4

(a) Top, representative immunostained images of astrocytes that were mock-infected, treated with DMSO or treated with 2 μM niclosamide, 92 μM PHA-690509, 9 μM emricasan, or a combination of 92 μM PHA-690509 and 9 μM emricasan for 1 h before infection with PRVABC59 (MOI = 0.5). Cells were fixed 24 h after infection and stained for ZIKVE (green) and nuclei (with DAPI; blue). Scale bar, 50 μm. Bottom, quantification of the percentage of ZIKV-infected astrocytes, relative to the number of DAPI-stained cells (n = 6 cultures). Values represent mean ± s.d. ***P < 0.001; by one-way ANOVA, as compared to DMSO-treated cells. (b) Top, representative western blot images of hNPCs that were treated with the indicated compounds and infected with PRVABC59 at a MOI of 0.1. Cells were analyzed 48 h after infection. Bottom, quantification of NS1 protein band intensities, relative to those of GAPDH (n = 3 cultures). Data were normalized to those for DMSO-treated cells. Values represent mean ± s.d. ***P < 0.01; by one-way ANOVA, as compared to DMSO-treated cells. (c) Virus production from compound-treated iPSC-derived human astrocytes (as in Fig. 2e) (n = 3 cultures). Data represent mean ± s.d. (d,e) Summary of the additive effects of treatment with a combination of emricasan and PHA-690509 on caspase-3 activity (d), as well as on improving cell viability as measured by ATP production (e), in human astrocytes infected with the FSS13025 (left) or MR766 (right) strain of ZIKV (n = 3). Values represent mean ± s.d. *P < 0.05; **P < 0.01; by one-way ANOVA.

Benefit of combining neuroprotective and antiviral compounds

Finally we explored combining these two categories of compounds (neuroprotective and antiviral). The two-drug combination of emricasan and PHA-690509 showed an additive effect in inhibiting caspase-3 activity in SNB-19 cells (Fig. 4d). A similar additive effect was found to preserve astrocyte viability after ZIKV infection (Fig. 4). Notably, emricasan did not interfere with PHA-690509's ability to inhibit ZIKV infection in the combination treatment (Fig. 4b and Supplementary Fig. 6a–c).

We also tested the effect of sequential treatment with the two categories of compounds. We found that treatment of PRVABC59-infected hNPCs with emricasan for 72 h followed by niclosamide treatment for 48 h led to the recovery of ZIKV-negative hNPCs, suggesting a beneficial effect of 'buying time' by inhibiting apoptosis to allow the infected cells to recover (Supplementary Fig. 6d).


Here we developed two ultra-high-throughput assays, using human neural cells, to measure ZIKV-induced caspase-3 activity and cell viability, and we screened over 6,000 approved drugs and drug candidate compounds. Our efforts so far have led to the identification of small molecules that either protect against cell death in multiple neural cell types or suppress ZIKV replication.

Emricasan, also called IDN-6556 or PF-03491390, is an inhibitor of activated caspases, and it has sub- to nanomolar activity in vitro48,49. Emricasan is currently being evaluated in phase 2 clinical trials for the reduction of hepatic injury and liver fibrosis caused by chronic HCV infection50,51. Emricasan was well tolerated in human trials, and there were no significant adverse events51. It was reported that overall and maximum concentrations of emricasan (orally, twice daily, ×4 d) in human blood were 1.90 μg/ml (3.35 μM) and 2.36 μg/ml (4.15 μM), respectively. Therefore, the reported human plasma concentration of emricasan is about tenfold higher than the IC50 for inhibition of increased caspase-3 activity and cell death caused by ZIKV infection in vitro. Future animal studies will be critical to evaluate the efficacy of emricasan in vivo. Whether it is safe to use emricasan during pregnancy for ZIKV infection in humans will need to be evaluated in preclinical toxicology studies and in clinical trials.

Ten structurally unrelated CDKis inhibit ZIKV replication and production, supporting a role for CDKs in the life cycle of ZIKV in human cells. Because flaviviruses are not known to encode any CDKs, these results suggest that one or more cellular CDKs in the host may be important for ZIKV replication. Further studies on target identification, including targeted kinome siRNA or CRISPR screens, may reveal additional insights into the mechanism of action for these inhibitors. Although many CDKis are being evaluated in clinical trials for various cancers, cystic fibrosis and Cushings disease, these compounds may not be suitable for pregnant women because of potentially hazardous effects on the fetus52. In our in vitro analyses, treatment with PHA-690509 or seliciclib partially rescued the ZIKV-induced reduction of hNPC proliferation, and the treatment with either compound in the absence of ZIKV infection showed a minimal effect on hNPC proliferation in brain organoid cultures, which model early human brain development in vitro (Supplementary Fig. 5c,d). Future studies in animal models, including both rodents and primates, are critical to test the efficacy and toxicity of identified compounds in vivo. Notably, these CDKis and their derivatives may be useful for treating nonpregnant humans who face an increased risk of Guillain–Barré syndrome and other conditions following ZIKV infection. For example, viral RNA and infectious virus have been detected in the semen of men months after acute symptoms have resolved53. In addition, these CDKis will be valuable chemical tools in probing the roles of specific types of CDKs in ZIKV infection, which could serve as new targets for anti-ZIKV drug development. The structural diversity of effective CDKis also provides multiple scaffolds for lead-compound optimization using medicinal chemistry.

Niclosamide is an FDA-approved drug (trade name Niclocide) that has been used in humans to treat worm infections for nearly 50 years, and it is well tolerated54,55. It is known to inhibit several viruses in culture systems, including the Japanese encephalitis flavivirus56,57,58. Its broad antiviral activity has been attributed to its ability to neutralize endolysosomal pH and interfere with pH-dependent membrane fusion57, which is an essential step in the common virus entry pathway. Our time-of-addition and time-course analyses, however, suggest that inhibition by niclosamide occurs at a post-entry step, such as replication. Future molecular studies of its mechanism of action may provide additional targets for drug development. Niclosamide is a category B drug, which indicates that no risk to fetuses has been found in animal studies. It has low toxicity in mammals with an oral median lethal dose (LD50) value of 5,000 mg per kg body weight (mg/kg) in rats59. The potency of niclosamide on inhibition of ZIKV replication is in the submicromolar range, whereas clinically it can be delivered at micromolar levels59. Additionally, a pro-drug formulation may further increase the bio-availability of this compound, which is currently indicated for treating intestinal parasites. The WHO recommends that niclosamide may be used during pregnancy because it has not been shown to be mutagenic, teratogenic or embryotoxic (http://apps.who.int/medicinedocs/en/d/Jh2922e/3.1.3.html). The US Centers for Disease Control and Prevention (CDC) concurs with the WHO recommendation and further recommends that “for individual patients in clinical settings, the risk of treatment (with Niclosamide) in pregnant women who are known to have an infection needs to be balanced with the risk of disease progression in the absence of treatment” (http://www.cdc.gov/parasites/hymenolepis/health_professionals/). Independently of evaluating the potential benefits and risks for pregnant women, niclosamide could be used to reduce viral load in infected men and nonpregnant women, which could reduce transmission and potentially prevent Guillain–Barré syndrome and other ZIKV-related complications in humans.

Despite rapid progress in the preclinical development of anti-ZIKV vaccines25,26, testing the safety and efficacy of vaccines in humans can take a substantial amount of time. Effective countermeasures against ZIKV, including small-molecule therapeutics, are also urgently needed. Our findings and the tools provided here should significantly advance current ZIKV research and have an immediate effect on the development of anti-ZIKV therapeutics. Furthermore, our findings could have implications for combating infections by other arboviruses, such as dengue viruses, chikungunya virus and West Nile virus, many of which can cause devastating illness.


Human forebrain-specific NPCs, astrocytes, organoids and cell line cultures.

The human iPSC line (C1-2 line) was previously generated from a skin biopsy sample of a healthy male newborn and has been fully characterized and passaged on mouse embryo fibroblast (MEF) feeder layers60. The BJ line was derived from healthy control fibroblasts obtained from the American Type Culture Collection (ATCC) (CRL-2522, male, neonatal). All studies followed institutional review board (IRB) protocols approved by Florida State University, Johns Hopkins University School of Medicine and Icahn School of Medicine at Mount Sinai. Human iPSCs were differentiated into forebrain-specific hNPCs following the previously established protocol60. Briefly, human iPSC colonies were detached from the feeder layer with 1 mg/ml collagenase treatment for 1 h and suspended in embryonic body (EB) medium, consisting of fibroblast growth factor (FGF)-2-free iPSC medium supplemented with 2 μM dorsomorphin (Sigma) and 2 μM A-83 (Tocris) in nontreated polystyrene plates for 4 d with a daily medium change. After 4 d, EB medium was replaced by neural induction medium (NPC medium), which consists of Dulbecco's modified Eagle's medium with F12 nutrient mixture (DMEM/F12), N2 supplement, non-essential amino acids (NEAA), 2 μg/ml heparin (Sigma) and 2 μM cyclopamine (Tocris). Floating EBs were then transferred to Matrigel-coated 6-well plates at day 7 to form neural-tube-like rosettes. Attached rosettes were kept for 15 d with an NPC medium change every other day. On day 22, rosettes were picked mechanically and transferred to low-attachment plates (Corning) to form neurospheres in NPC medium containing B27 supplements (Invitrogen). Neurospheres were then dissociated with Accutase (Millipore) at 37 °C for 10 min and placed onto Matrigel-coated 6-well plates at day 24 to form monolayer hNPCs in NPC medium containing B27. These hNPCs expressed forebrain-specific progenitor markers60, including NESTIN, PAX6, EMX-1, FOXG1 and OTX2.

Human BJ iPSC line and forebrain NPCs were derived as described previously61,62. Human iPSC-derived forebrain NPCs were maintained at high density, grown on Matrigel (BD Bioscience) in medium consisting of DMEM/F12, 1× N2, 1× B27-RA (Invitrogen), 1 μg/ml laminin (Invitrogen) and 20 ng/ml FGF-2 (Invitrogen). hNPCs were differentiated to astrocytes and cultured on Matrigel-coated plates in astrocyte medium (ScienCell). Astrocytes were split 1:3 every week with Accutase (Millipore) and cultured up to 120 d.

Forebrain-specific organoids were generated from the C1-2 human iPSC line as previously described17. Briefly, on day 1, human iPSC colonies were detached 7 d after passage with collagenase type IV (Thermo Fisher Scientific), washed with fresh stem cell medium and transferred to an ultra-low-attachment 6-well plate (Corning Costar), containing 3 ml of stem cell medium (without FGF-2), plus 2 μM dorsomorphine and 2 μM A83-01. On days 5–6, half of the medium was replaced with induction medium consisting of DMEM/F12, 1× N2 supplement (Invitrogen), 10 μg/ml heparin, 1× penicillin–streptomycin, 1× NEAA, 1× Glutamax, 4 ng/ml WNT-3A (R&D Systems), 1 μM CHIR99021 (Cellagentech) and 1 μM SB-431542 (Cellagentech). On day 7, organoids were embedded in Matrigel (BD Biosciences) and continued to grow in induction medium for 6 more days. On day 14, embedded organoids were mechanically dissociated from Matrigel by pipetting up and down onto the plate with a 5-ml pipette tip. Typically, 10–20 organoids were transferred to each well of a 12-well spinning bioreactor (SpinΩ) containing differentiation medium, consisting of DMEM/F12, 1× N2 and B27 supplements (Invitrogen), 1× penicillin–streptomycin, 1× 2-mercaptoenthanol, 1× NEAA and 2.5 mg/ml insulin (Sigma). Day 18 forebrain organoids were exposed to ZIKV FSS-13025 in SpinΩ for 24 h and then in replaced fresh medium for an additional 9 d before fixation and immunostaining as previously described17. To test the potential toxic effect on hNPC proliferation, day 20 forebrain organoids were also treated with PHA-690509 (1 μM) or seliciclib (5 μM) for 3 d without ZIKV exposure. On day 23 (20 + 3), treated forebrain organoids were pulsed with 10 μM 5-ethynyl-2-deoxyuridine (EdU; Thermo Fisher Scientific) for 1 h and immediately fixed for analysis.

The glioblastoma SNB-19 cell line (part of the National Cancer Institute 60 human tumor cell lines) was a gift from Dr. David Meckes (Florida State University, Tallahassee, FL). SNB-19 cells were maintained at 37 °C in 5% CO2 in RPMI-60 medium, 1× penicillin–streptomycin and 10% FBS (Invitrogen). The Aedes albopictus C6/36 cell line (ATCC) was maintained at 28 °C in 5% CO2.

Preparation of ZIKV and cell infection.

The MR766-ZIKV stock with the titer of 1 × 105 tissue-culture-infective dose (TCID)/ml, in the form of culture fluid from an infected rhesus Macaca cell line LLC-MK2, was originally obtained from ZeptoMetrix (Buffalo, NY). The FSS13025-ZIKV strain was obtained from Drs. Robert Tesh and Pei-Yong Shi (University of Texas Medical Branch, Galveston, Texas). The PRVABC59 strain was obtained from ATCC (Manassas, VA). Original viral stocks were then amplified in Aedes albopictus clone C6/36 cells. Briefly, C6/36 cells were inoculated with viral inoculum for 1 h at 28 °C in a low volume of medium (3 ml per T-75 flask), with rocking every 15 min, before the addition of 17 ml medium. Virus-inoculated cells were incubated at 28 °C for 6–7 d before harvesting the supernatant. C6/36-amplified ZIKV titer was determined by infecting Vero cells for 48 h with a methylcellulose overlay and analyzed for focus-forming units per ml (FFU/ml). In mock infections, an equal volume of spent uninfected C6/36 culture medium was used. For infections, cells were seeded into 12-well plates 1 d before virus addition. For all cell types, compound was added 1 h before viral addition unless otherwise specified. Cells were harvested at 24–72 h after infection.

Compound libraries.

The Library of Pharmacologically Active Compounds (LOPAC), which consists of 1,280 compounds, was purchased from Sigma-Aldrich. The NCATS pharmaceutical collection63, a collection consisting of 2,816 clinically approved and investigational drugs, was established in 2011. All compounds were dissolved in DMSO as 10-mM stock solutions, then diluted in DMSO at a 1:3 ratio in 384-well plates, followed by reformatting into 1,536-well compound plates for use in high-throughput screening (HTS).

Caspase-3 assay.

Caspase-Glo 3/7 assay kit (catalog number G8092; Promega, Madison, WI) was used to detect caspase-3 activity. Reagents were reconstituted as described in the protocol from the manufacturer. Polystyrene plates (384-well and 1,536-well; regular tissue-culture-treated and PDL-coated) were purchased from Greiner Bio-One (Monroe, NC). Cells were seeded in 384- and 1536-well assay plates and cultured at 37 °C with 5% CO2 for 16 h. ZIKV solution was added to cells, followed by incubation at 37 °C with 5% CO2 for 6 h. Caspase-Glo-3/7 reagent was added to each well, unless otherwise specified, and incubated at room temperature for 30 min. The luminescence intensity of the assay plates was measured using a ViewLux plate reader (PerkinElmer). Data were normalized by using the cell-containing wells without ZIKV as a negative control (0% induction of caspase-3 activity) and wells containing ZIKV infected cells that induced caspase-3 activity were used as a positive control (100% induction of caspase 3 activity).

ATP content assay for cell viability and compound cytotoxicity.

The ATPlite luminescence assay system assay kit (catalog number 6016731; PerkinElmer) was used to determine cell viability. The reagent was reconstituted and prepared as described by the manufacturer. In order to measure the cell death caused by ZIKV infection, cells were cultured for 16 h at 37 °C with 5% CO2 in assay plates, followed by addition of ZIKV solution and incubation at 37 °C with 5% CO2 for 72 h. ATPlite, the ATP-monitoring reagent, was then added to the assay plates, which were then incubated for 15 min. The resulting luminescence was measured using the ViewLux plate reader. Data were normalized using wells without cells as a control for 100% cell killing, and cell-containing wells without ZIKV infection as full cell viability (0% cell killing). For analysis of potential toxicity of select compounds, cells were seeded in 96-well plates. One day later, cells were treated with the indicated compounds and concentrations for 24–48 h before the addition of Cell Titer-Glo substrate (Promega) and measurement, according to manufacturer's instructions.

Large-scale compound screening.

A quantitative high-throughput screening (qHTS, ref. 64), in which each compound was assayed in four concentrations (0.37, 1.84, 9.2 and 46 μM), was performed in singlet for the primary compound screen. While a single-compound concentration (in singlet) has been traditionally used for HTS of large compound collections (such as 1 to 3 million compounds), the qHTS format with multiple compound concentrations has recently been used for medium or small compound collections, such as an approved drug library. Specifically, SNB-19 cells and hNPCs were seeded onto PDL-coated 1,536-well assay plates at 250 cells per 3 ml per well and incubated at 37 °C in 5% CO2 for 16 h. Test compounds, dissolved in DMSO, were transferred to assay plates at a volume of 23 nl/well by an automated pintool workstation (Wako Automation, San Diego, CA). Compounds were incubated with cells for 30 min at 37 °C in 5% CO2, immediately followed by the addition of 2 ml/well of ZIKV (2 FFU/cell). Incubation time of compound-treated cells with ZIKV varied based on assay format. Experiments measuring virus-induced caspase-3/7 activity required a 6-h incubation of ZIKV in the presence of compounds at 37 °C in 5% CO2. Following this incubation, 3.5 μl/well of caspase-3/7 reagent mixture was added to the assay plates. The plates were incubated for 30 min at room temperature, and the resultant luminescence signal was measured using a ViewLux plate reader (Perkin Elmer). Experiments measuring virus-induced cell death required a 72-h incubation of ZIKV in the presence of the compounds, at 37 °C in 5% CO2. Following this incubation, 3.5 μl/well of ATP content detection reagent was added to assay plates. The plates were incubated for 30 min at room temperature, and the resultant luminescence signal was measured in a ViewLux plate reader. Step-by-step assay protocols are listed in Supplementary Tables 1 and 2.

Confirmation of primary hits and counter-screen.

The primary hits were selected with criteria of IC50 values ≤ 30 μM, and maximal inhibition ≥ 50%. The hit compounds were diluted 1:3 in DMSO to 11 concentrations for the confirmation experiments. The same caspase-3 activity assay was first used to confirm the activity of the primary-hit compounds (n = 3). In order to further confirm the activity of these compounds, the protective effect of these primary hits on the cell death caused by incubation of cells with ZIKV for 3 d was also determined using an ATP content cell viability assay (n = 3).

Because compound cytotoxicity could nonspecifically reduce the caspase activity induced by ZIKV, we also used the ATP content assay to measure compound cytotoxicity in the absence of ZIKV infection. Cells were seeded in the same way as described above in 1,536-well assay plates. After a 6-h incubation with compounds in the absence of ZIKV, 3.5 μl/well of ATP content reagent mixture was added to the assay plates, which were then incubated for 30 min at room temperature. The luminescence signal in the assay plates was measured using a ViewLux plate reader (Supplementary Table 3). Any compounds that exhibited cytotoxicity were eliminated as false-positive compounds.

Western blot analysis.

Cells were harvested by trypsinization, pelleting and subsequent lysis in 1× Laemlli buffer, and the lysates were then boiled, or the cells were directly lysed in 1× Laemlli buffer and boiled. Antibodies used were anti–ZIKV NS1 (1:2,000; BF-1225-36, BioFront Technologies, Tallahassee, FL) or anti-GAPDH (sc-25778, Santa Cruz Biotechnology, Texas). The screening of two subsets of compounds for antiviral activity (Supplementary Fig. 2a and Supplementary Fig. 4b) was performed in a blinded manner, whereas all other experiments were performed in a nonblinded manner.


Cells were fixed with 4% paraformaldehyde (Sigma) for 15 min at room temperature. Samples were permeabilized and blocked with 0.25% Triton X-100 (Sigma) and 10% donkey or goat serum in phosphate-buffered saline (PBS) for 20 min as previously described60. Samples were then incubated with primary antibodies at 4 °C overnight, followed by multiple PBST (PBS plus Tween-20) washes and incubation with secondary antibodies for 1 h at room temperature. Slides were mounted using VECTASHIELD with 4′,6-diamidino-2-phenylindole (DAPI; Vectorlabs, Burlingame, CA). The following primary antibodies were used: anti–flavivirus group antigen (clone D1-4G2-4-15; mouse; 1:500; Millipore), anti–cleaved caspase-3 (Asp15; rabbit; 1:500; Cell Signaling Technology) and anti–phospho-histone-H3 (PH3; 9701S; rabbit; 1:300; Cell Signaling Technology) as previously described17. Antibodies were prepared in PBS containing 0.25% Triton X-100 and 10% donkey serum. For EdU assay, the Click-iT EdU Alexa Fluor 488 Imaging Kit (Thermo Fisher Scientific) was used according to the manufacturer's protocol. Images were taken by Zeiss LSM 700 and 880 confocal microscopes, an Olympus BX61 microscope or a Zeiss Axiovert 200M microscope.

For organoid studies, quantitative analyses were conducted on randomly selected cortical structures captured by confocal microscope in a blinded fashion (example as shown in Fig. 1c). Cell death and cell proliferation were quantified by counting activated caspase-3+ and PH3+ nuclei, respectively, relative to the total number of nuclei stained by DAPI in the ventricular structures in at least six samples, as previously described17. We determined our sample sizes based on previous studies conducted in our lab17.

NS1 enzyme-linked immunosorbent assay (ELISA).

The anti-ZIKV NS1 ELISA kit (ZKV-NS1-EK) was obtained from BioFront Technologies (Tallahassee, FL) and used according to the manufacturer's protocol.

Viral titer by focus-forming unit (FFU) assay.

ZIKV titers from cell supernatants were determined by infecting Vero cells for 48 h with a methylcellulose overlay and analyzing the plates for focus-forming units per ml (FFU/ml). Briefly, cell supernatant was titrated in triplicates onto a monolayer culture of Vero cells in 96-well plates and incubated at 37 °C for 2 h. Virus inoculum was removed and replaced with a methylcellulose overlay. Vero cells were incubated for an additional 48–72 h before fixation and incubated with anti–flavivirus group antigen overnight at 4 °C. The next day, fixed cells were washed three times with PBS and incubated with horseradish peroxidase (HRP)-conjugated anti-mouse secondary antibody for 1 h at room temperature, washed again three times with PBS and incubated with DAB peroxidase substrate for 10 min (Vector Labs).

Antiviral compound analysis.

SNB-19 cells, human astrocytes or hNPCs were seeded in 12-well plates at approximately 3 × 105 cells/well. The next day, cells were treated with compound at 1- to 10-fold of the IC50 value, or the indicated concentration, for 1 h before inoculation with ZIKV (multiplicity of infection (MOI) = 0.5–1). Cells and supernatant were harvested 24–48 h post infection and analyzed by western blot, immunostaining or quantitative RT–PCR analyses. Western blot bands were quantified, and immunostaining images were counted using ImageJ (NIH, Bethesda, MD). For qRT–PCR analysis, total cellular RNA was purified using the RNeasy Mini Plus kit (Qiagen). About 500–1,000 ng total RNA was reverse-transcribed into cDNA using random hexamers according to manufacturer's instructions (Superscript III First Strand Synthesis System, Invitrogen). Quantitative PCR was performed using SYBR Green PCR master mix (Invitrogen), gene specific primers (ZIKV-NS1-Forward: TGGAGTTCAACTGACGGTCG; ZIKV-NS1-Reverse: TACCCCGAACCCATGATCCT; Gapdh-Forward: TCACTGCCACCCAGAAGACTG; and Gapdh-Reverse: GGATGACCTTGCCCACAGC), and an Applied Biosystems 7500 Fast real-time PCR system. A 60 °C to 95 °C melt curve analysis following PCR was performed using default settings. Relative quantification was performed using the ΔΔCT method with Gapdh as the endogenous control, and the relative fold change was calculated by normalizing to the levels in the control cells.

Data analysis and statistics.

The primary-screen data and concentration response curves were analyzed using software developed internally65. The IC50 values of compound confirmation data were calculated using the Prism software (GraphPad Software, Inc. San Diego, CA). All values are expressed as the mean ± s.d. unless specified otherwise. Western blots were quantified using ImageJ (NIH, Bethesda, MD). We did not exclude any samples. Experiments were not blinded, except for those that were specified. The sample sizes were estimated according to previous studies and the known variability of the assays. Statistical analyses were carried out with the one-way ANOVA using the Prism software. The Z′ factor, a measure of statistical effect size and an index for assay quality control, was calculated by: Z′ = 1 − ((3 × s.d.signal) + (3 × s.d.basal)/(Meansignal − Meanbasal)).

Accession codes.

PubChem Bioassay Database: all of the results from the primary screen of the approved drug collection and hit confirmation were deposited under assay IDs 1224859, 1224857, 1224858, 1224853, 1224855, 1224861, 1224862, 1224860, 1224856, 1224854 and 1224852.



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We thank R. Tesh and P.-Y. Shi (University of Texas Medical Branch) and the World Reference Center for Emerging Viruses and Arboviruses (WRCEVA) for the FSS-13025 isolate of ZIKV, and D. Meckes (Florida State University) for the glioblastoma SNB-19 cell line. We also thank L. Liu and Y. Cai for technical support. This work was supported by the Intramural Research Program of the National Center for Advancing Translational Sciences, National Institutes of Health (NIH) (W.Z.), ZIKV seed funding from Florida State University (H.T.), a start-up fund from Emory University (Z.W.), the Brain and Behavior Research Foundation (K.J.B.), the New York Stem Cell Foundation (K.J.B.), the Maryland Stem Cell Research Fund (G.M. and H.S.), the Simons Foundation Autism Research Initiative (award no. 308988; H.S.), and partially by NIH grants NS048271 (G.M.), NS095348 (G.M.), MH105128 (G.M.), NS047344 (H.S.), NS097206 (H.S.), MH106434 (H.S.), MH101454 (K.J.B.), MH106056 (K.J.B.), AG005138 (K.J.B.), AG046170 (K.J.B.) and AI119530 (H.T.).

Author information

Author notes

    • Miao Xu
    • , Emily M Lee
    •  & Zhexing Wen

    These authors contributed equally to this work.

    • Guo-li Ming
    • , Wei Zheng
    • , Hongjun Song
    •  & Hengli Tang

    These authors jointly directed this work.


  1. National Center for Advancing Translational Sciences, National Institutes of Health, Bethesda, Maryland, USA.

    • Miao Xu
    • , Jennifer Kouznetsova
    • , Misha Itkin
    • , Paul Shinn
    • , Samuel G Michael
    • , Anton Simeonov
    • , Wenwei Huang
    • , Ruili Huang
    • , Menghang Xia
    •  & Wei Zheng
  2. Sir Run Run Shaw Hospital, Zhejiang University School of Medicine, Hangzhou, China.

    • Miao Xu
  3. Department of Biological Science, Florida State University, Tallahassee, Florida, USA.

    • Emily M Lee
    • , Yichen Cheng
    • , Sarah C Ogden
    • , Christy Hammack
    • , Catherine Hanna
    • , Chase Allen
    •  & Hengli Tang
  4. Department of Psychiatry and Behavioral Science, Emory University School of Medicine, Atlanta, Georgia, USA.

    • Zhexing Wen
  5. Department of Cell Biology, Emory University School of Medicine, Atlanta, Georgia, USA.

    • Zhexing Wen
  6. Department of Neurology, Emory University School of Medicine, Atlanta, Georgia, USA.

    • Zhexing Wen
  7. Institute for Cell Engineering, Johns Hopkins University School of Medicine, Baltimore, Maryland, USA.

    • Zhexing Wen
    • , Wei-Kai Huang
    • , Xuyu Qian
    • , Fadi Jacob
    • , Ha Nam Nguyen
    • , Kimberly M Christian
    • , Guo-li Ming
    •  & Hongjun Song
  8. Department of Pathology, Johns Hopkins University School of Medicine, Baltimore, Maryland, USA.

    • Wei-Kai Huang
  9. Biomedical Engineering Graduate Program, Johns Hopkins University School of Medicine, Baltimore, Maryland, USA.

    • Xuyu Qian
    • , Guo-li Ming
    •  & Hongjun Song
  10. Department of Neuroscience, Icahn School of Medicine at Mount Sinai, New York, New York, USA.

    • Julia TCW
    •  & Alison Goate
  11. The Solomon H. Snyder Department of Neuroscience, Johns Hopkins University School of Medicine, Baltimore, Maryland, USA.

    • Fadi Jacob
    • , Guo-li Ming
    •  & Hongjun Song
  12. Department of Neurology, Johns Hopkins University School of Medicine, Baltimore, Maryland, USA.

    • Ha Nam Nguyen
    • , Kimberly M Christian
    • , Guo-li Ming
    •  & Hongjun Song
  13. Department of Psychiatry, Icahn School of Medicine at Mount Sinai, New York, New York, USA.

    • Kristen J Brennand
  14. Department of Psychiatry and Behavioral Sciences, Johns Hopkins University School of Medicine, Baltimore, Maryland, USA.

    • Guo-li Ming
  15. The Kavli Neuroscience Discovery Institute, Johns Hopkins University School of Medicine, Baltimore, Maryland, USA.

    • Guo-li Ming
    •  & Hongjun Song


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M. Xu, E.M.L., Z.W., A.S., K.M.C., M. Xia, G.M., W.Z., H.S. and H.T. conceived of the research, designed the study, interpreted data and wrote the manuscript; M. Xu, E.M.L., Z.W., Y.C., W.-K.H., X.Q., J.K., S.C.O., C. Hammack, F.J., H.N.N., M.I., C. Hanna, P.S., C.A., S.G.M. and W.H. performed experiments; J.T., A.G. and K.J.B. provided astrocytes; R.H. analyzed data; G.M., W.Z., H.S. and H.T. are co-senior authors who directed the research.

Competing interests

The authors declare no competing financial interests.

Corresponding authors

Correspondence to Guo-li Ming or Wei Zheng or Hongjun Song or Hengli Tang.

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