Rapid identification of host genes essential for virus replication may expedite the generation of therapeutic interventions. Genetic screens are often performed in transformed cell lines that poorly represent viral target cells in vivo, leading to discoveries that may not be translated to the clinic. Intestinal organoids are increasingly used to model human disease and are amenable to genetic engineering. To discern which host factors are reliable anti-coronavirus therapeutic targets, we generate mutant clonal IOs for 19 host genes previously implicated in coronavirus biology. We verify ACE2 and DPP4 as entry receptors for SARS-CoV/SARS-CoV-2 and MERS-CoV respectively. SARS-CoV-2 replication in IOs does not require the endosomal Cathepsin B/L proteases, but specifically depends on the cell surface protease TMPRSS2. Other TMPRSS family members were not essential. The newly emerging coronavirus variant B.1.1.7, as well as SARS-CoV and MERS-CoV similarly depended on TMPRSS2. These findings underscore the relevance of non-transformed human models for coronavirus research, identify TMPRSS2 as an attractive pan-coronavirus therapeutic target, and demonstrate that an organoid knockout biobank is a valuable tool to investigate the biology of current and future emerging coronaviruses.
Three highly pathogenic coronaviruses have spread to humans in the past two decades. The Severe Acute Respiratory syndrome coronavirus (SARS-CoV) emerged in 2002 and rapidly spread between continents, but was controlled by public health interventions. Middle East respiratory syndrome virus (MERS-CoV) -discovered in 2012- causes an ongoing outbreak in the Middle East with a high case-fatality ratio of 35%, but has not attained efficient human-to-human transmission. The latest, SARS-CoV-2, emerged at the end of 2019 and is the causative agent of the COVID-19 pandemic1. While vaccine development has taken off at a tremendous pace, drugs that target either the virus or host factors essential for virus replication have been more difficult to develop as this requires a deep understanding of coronavirus biology.
The first step in coronavirus replication is the attachment to host cells, which is dependent on the viral spike glycoprotein2. Although (proteo)glycans are often involved in the initial attachment, most coronavirus spikes require a specific transmembrane protein for entry. After receptor engagement, the next step in viral entry involves proteolytic cleavage of the spike protein. This cleavage step is performed by host proteases and destabilizes the spike, causing a conformational change and the subsequent fusion of viral and host membranes. This releases the viral ribonucleoprotein complex into a host cell and initiates replication.
Most of what we know on coronavirus cell biology stems from studies on 2D transformed cell lines such as the Vero E6 kidney cell line, derived from an African green monkey3. Work on cell lines has identified ACE2 as the entry receptor of SARS-CoV-2 and SARS-CoV, and DPP4 as the entry receptor of MERS-CoV4,5,6. Cell lines typically consist of a homogeneous population of poorly differentiated cells, potentially limiting the translatability of findings. As a case in point, chloroquine, an endocytosis inhibitor, has been proposed as a SARS-CoV-2 antiviral drug as it blocks SARS-CoV-2 entry in several cell lines7, yet clinical studies have failed to demonstrate efficacy in COVID-19 patients8. Along these lines, inhibiting protease groups in cell lines with relatively broad-acting inhibitors have revealed that spike protein cleavage can occur at the cell surface by transmembrane serine protease (e.g., TMPRSS family members) or in the endosome by cathepsins (e.g., Cathepsin B or L), depending on the cell line used. Recently published host gene loss-of-function screens in 2D cell lines have supported a role for Cathepsin L, but not TMPRSS2, in viral entry into VeroE6 cells, while the opposite was observed in a small scale CRISPR screen Calu-3 cells9,10. In addition, we and others have recently shown that in primary airway cells serine protease- (but not cathepsin-) inhibitors block viral entry4,11, but these inhibitors target all TMPRSS family members. Thus, it remains unknown whether in primary cells TMPRSS2 would be a realistic therapeutic target, or whether other TMPRSS family members could compensate for the loss of TMPRSS2. Similarly, several new host factors have recently been found to play a role in the SARS-CoV-2 replication cycle, such as NRP1 and NDST1, but it is unknown whether these genes could be used as anti-SARS-CoV-2 drug targets12,13,14.
There may exist significant differences between individual transformed cell lines, and between transformed and non-transformed cells in viral entry pathways. Intestinal organoid (IO) culture systems are an attractive platform to study virus-host interactions as they are amenable to CRISPR-Cas9 mediated gene editing to directly identify host proteins utilized by the virus. Their self-renewing nature offers an additional advantage: biobanks of characterized mutant IO clones can be established, stored and shared. In this work, we establish a biobank of mutant IOs in genes implied in coronavirus biology and test their role in coronavirus replication to discern which host factors may represent anti-coronavirus therapeutic targets. This biobank can be used as a tool to rapidly identify which genes are essential for virus entry when novel SARS-CoV-2 variants or novel zoonotic (corona)viruses emerge.
Transcriptomic analysis of human IOs and airway cultures reveal conserved expression of coronavirus host factors
Multiple host factors such as entry receptors and proteases are involved in viral replication cycles15. Since organoids closely resemble the physiology of human tissues, we used IOs to assess the function of individual host factors that have been implicated in the SARS-CoV-2 replication cycle, or of other coronaviruses. We and others have previously shown that SARS-CoV-2 can replicate in human IOs16,17,18, consistent with observations of gastrointestinal symptoms in COVID-1919,20. Intestinal organoids are readily amenable to genetic engineering by CRISPR-Cas921, allowing to test the role of host genes in the replication of SARS-CoV-2. We reasoned that individual host factors that upon loss-of-function affect coronavirus replication, represent interesting drug targets for the treatment of COVID-19. As spike protein cleavage is an essential step for viral entry, we focused on the proteases TMPRSS2, TMPRSS3, TMPRSS4, TMPRSS11D, TMPRSS13, Cathepsin B (CTSB), Cathepsin L (CTSL) and Furin, that have previously been implicated in the entry of SARS-CoV-2 or other coronaviruses9,22,23. Besides proteases, we included the following (putative) entry or attachment factors: the protease DPP4 (MERS-CoV), peptidase ANPEP (human coronavirus 229E receptor24, C-type lectin CLEC2B25, structural protein Vimentin26, glycoprotein CEACAM127, tetraspanin CD928, C-type lectin receptor CD209 (DC-SIGN)29, VEGF co-receptor NRP113,14, MAVS which indirectly senses cytoplasmic RNA30, heatshock protein HSPA531, the sulfotransferase NDST112 and the RNA packaging protein ARC (upregulated upon SARS-CoV-2 infection17, Fig. s6e) as putative host factors involved in replication.
We first confirmed the expression of these host factors in human IOs using a previously generated dataset (Fig. 1a, s1a)17. To extend the expression analysis, we performed single cell RNA sequencing of expanding and differentiated IOs to assign host factors to individual cell types. The organoid atlas was supplemented by a recently published intestinal tissue dataset which we reanalyzed to allow for direct comparison32. Cells grouped into distinct stem cell, progenitor, goblet cell and enterocyte clusters (Fig. s1b–d). The proteases were ubiquitously expressed among the different lineages, with the exception of TMPRSS2 which displayed a slight bias towards enterocytes, and TMPRSS4 that was enriched in undifferentiated cells in both tissue and organoids (Fig. 1b). These findings contrasted with a recent study that used murine tissue data and identified goblet-cell enriched expression of TMPRSS2, while TMPRSS4 was mostly found in enterocytes33.
We additionally performed RNA sequencing of 3D nasal organoids and 2D air-liquid interface differentiated airway organoids, confirming expression of all selected host genes in these epithelia, while relative expression levels varied (Fig. 1a, S1A, Supplementary Dataset 1). Of note, the airway proteases TMPRSS11A and TMPRSS11D were expressed in lower airway cultures, while expressed to modest levels in IOs and nasal epithelial organoids (Fig. 1a, s1a).
ACE2 is the obligate entry receptor of SARS-CoV and SARS-CoV-2
Having established expression of key coronavirus host factors, we generated an extensive biobank of IOs harboring a loss-of-function mutation in individual genes (Figs. 2a, s2–3). We employed transient transfection of a Cas9-EGFP encoding plasmid that included a site-specific guide RNA (sgRNA). Transfected cells were GFP-sorted to establish clonal lines (12–24 lines per gene), expanded and sequenced to identify loss-of-function clones. We successfully established 2–6 mutated clonal IO cultures for all genes with the exception of HSPA5 (0 lines) and Furin and ARC (1 line) (Fig. 2b, Dataset 2). HSPA5 is a heatshock protein that was recently identified as an essential gene for cell survival34.
We first focused on ACE2, generally accepted to be the entry receptor for SARS-CoV-2 and SARS-CoV, as based on crystallographic evidence and overexpression studies5. Moreover, transgenic mice expressing human ACE2 are susceptible to infection with the virus35. Multiple additional (co-)receptors have been proposed for SARS-CoV-2, including CD209/DC-SIGN, and NRP113,14,36. Recent findings in human IOs have found no correlation between infectability of cells and their levels of ACE2 expression, suggesting the potential existence of alternative entry receptors37. In line with these findings, we observed both ACE2-positive and ACE2-negative SARS-CoV-2 infected cells in IOs (Fig. s4), although absence of surface-ACE2 could also indicate downregulation after infection37 or reflect expression levels under the detection limit of immunofluorescence staining.
To unequivocally demonstrate that physiological levels of ACE2 are essential for SARS-CoV-2 entry into non-transformed human epithelial cells, we analyzed mutant ACE2 IOs for their ability to support SARS-CoV-2 replication. ACE2, located on the apical membrane of cells in wildtype IOs, was lost in mutant clones (Fig. 2c). ACE2-deficient IOs were fully resistant to SARS-CoV-2 infection (Fig. 3a). Indeed, we did not detect SARS-CoV-2 infected cells in ACE2-knockout organoids by immunofluorescence (Fig. 3b). Similarly, infection with SARS-CoV was abrogated in ACE2-knockout organoids (Fig. s5a). We concluded that ACE2 is the obligate entry receptor for SARS-CoV-2 and SARS-CoV, and that no redundancy exists with other surface proteins in intestinal epithelial cells. The presence of infected cells that appear ACE2-negative, implies either that surface receptors are downregulated upon infection or that low levels of ACE2 proteins suffice. To confirm that viral entry occurs through the apical membrane—where ACE2 is located—we attempted viral infection following our standard approach in which organoids are mechanically disrupted, and using intact organoids where only the basolateral surface is exposed. We could observe viral replication only in disrupted organoids, supporting an obligate apical entry route for SARS-CoV-2 (Fig. s5b).
MERS-CoV infects human IOs in a DPP4-dependent manner
DPP4 has been shown to be the entry receptor for MERS-CoV by spike co-immunoprecipitation and overexpression in non-susceptible cells6. We first established that human IOs allow replication of MERS-CoV (Fig. s6a). In contrast to SARS-CoV-2, MERS-CoV caused extensive cell death, killing the majority of cells in organoids within 48 h of infection (Fig. s6a). Transcriptomic analysis revealed a strong upregulation of heat shock- and unfolded protein responses, while interferons were effectively repressed (Fig. s6b–e, Supplementary Datasets 3–4). This was consistent with previous reports that MERS-CoV encodes an extensive set of proteins that inhibit interferon responses38. We generated loss-of-function DPP4-mutant IO clones (Supplementary dataset 2). An infection assay on two of these clones revealed that MERS-CoV replication was fully blocked, while SARS-CoV-2 replicated in the DPP4-mutant organoids at control levels (Fig. 3c). Immunofluorescence confirmed loss of DPP4 protein in mutant clones as well as the successful replication of SARS-CoV-2 -but not of MERS-CoV- in these organoids (Fig. 3d). Conversely, MERS-CoV propagated in ACE2-deficient organoids at control levels (Fig. s5a).
Loss-of-function screen of host proteases reveals essential role in viral replication for TMPRSS2 but not other TMPRSS family members or Cathepsins
We next analyzed all IO lines that were mutant in proteases for their ability to support SARS-CoV-2 replication. Knockout of TMPRSS2 effectively blocked viral replication, while mutation of any of other TMPRSS-genes or cathepsins had no effect (Fig. 4a, b). Complete depletion of TMPRSS2 protein was confirmed using immunohistochemistry (Fig. s7a). These experiments were performed using a VeroE6-propagated stock and recent work has pointed out that propagation on VeroE6 cells can lead to culture adaptive mutations in the multibasic cleavage site39,40,41,42,43. The VeroE6 stock used in this study was deep-sequenced39 and was 64.2% wild-type in the RRAR (spike positions 682–685) multibasic cleavage site. We detected another mutation adjacent to the multibasic cleavage site (S686G) at a frequency of 45.4%. Viruses with multibasic cleavage site cleavage site mutations, including S686G, were shown to increase cathepsin usage in cells that contained both the cathepsin and serine protease-mediated entry pathway39. Despite the presence of variants in this SARS-CoV-2 stock, replication was not affected by the deletion of cathepsins.
We have previously shown that propagation in TMPRSS2-expessing Calu-3 cells prevents culture adaptation. Using this Calu-3 stock that was completely non-adapted39, we confirmed the dependency of SARS-CoV-2 on TMPRSS2 (and ACE2), but not CTSL (Fig. 4c). Immunofluorescence of TMPRSS2-deficient organoids showed absence of viral spread (Fig. 4d). This implied that TMPRSS2 is the main proteolytic activator of the authentic SARS-CoV-2 spike protein. In contrast to knockout screens in VeroE6 cells that showed that the endocytic pathway protease Cathepsin L was essential for SARS-CoV-2 entry9, SARS-CoV-2 replicated -if anything- more efficiently in Cathepsin L-mutant than in wildtype organoids (Fig. 4a, b). Efficient depletion of Cathepsin L was supported using western blot analysis (Fig. s7b). We confirmed the obligate role of TMPRSS2 for SARS-CoV-2 replication in IOs derived from a different donor and from another segment (duodenum) of the human intestine (Fig. 4e).
Since we observed differential expression of multiple proteases—including upregulation of cathepsins—in differentiated organoids, we additionally assessed TMPRSS2-dependency in differentiated intestinal cells (Fig. s7c). After 5 days of differentiation, both wildtype and TMPRSS2-mutant organoids were infected with SARS-CoV-2. SARS-CoV-2 replicated efficiently in differentiated organoids, as we reported previously17. Viral replication was greatly diminished in TMPRSS2-deficient organoids, suggesting dependency on this protease across different intestinal cell types (Fig. s7d).
To assess redundancy in single TMPRSS- or cathepsin-mutant organoids, we additionally generated organoids mutant for both CTSL/CTSB, or TMPRSS2/4, the most abundantly expressed cathepsins and serine proteases in the intestinal epithelium. Previous work implied a role for TMPRSS4 in viral entry in the intestinal epithelium33. We did not observe reduced replication when both cathepsins were lost. Moreover, TMPRSS4 knock-out in a TMPRSS2-mutant background did not further decrease infectivity (Fig. s7e). In line with this, the broad serine protease inhibitor camostat did not affect replication in TMPRSS2-deficient IOs (Fig. s7f). We concluded that the cathepsins and TMPRSS4 do not play a role in viral entry in the intestinal epithelium.
To confirm that the endocytic pathway is dispensable for viral entry, we treated IOs with the endosomal pathway inhibitor chloroquine, the cathepsin protease inhibitor E64D, or the broad serine protease inhibitor camostat. These drugs were well-tolerated with no growth impairment at the concentrations used (Fig. s8a, b). As published previously, chloroquine was effective in VeroE6 cells (Fig. s8c)7. While camostat effectively inhibited viral replication, chloroquine and E64D did not affect replication in IOs (Fig. 4f). E64D-treated organoids displayed a trend towards more efficient viral replication (Fig. 4f), consistent with observations in the Cathepsin L-mutant organoids (Fig. 4a, b). We concluded that Cathepsin-mediated entry through the endosomal route may be the central port of viral entry in some cell lines, but not in IOs, in which SARS-CoV-2 enters through the activity of TMPRSS2 (Fig. 4a, b). These observations may also explain why (hydro)-chloroquine has emerged from cell line studies but has proven ineffective in the clinic.
Redundancy for non-protease host factors in viral replication
We further tested IOs mutant in a range of non-protease host factors to assess their role in coronavirus replication, of which some have already been linked to the SARS-CoV-2 replication cycle. NRP1 recently attracted attention as a novel co-receptor for SARS-CoV-2 in two separate studies that used Hela, HEK293T and the colorectal cancer cell line Caco-213,14. These findings were substantiated by x-ray crystallography data supporting binding of the viral spike protein to NRP1 SARS-CoV-2 infection was significantly inhibited by NRP1-blocking antibodies13,14. In addition, CD209 was recently identified as potential SARS-CoV-2 receptor, and facilitated viral entry in HEK-293 cells when overexpressed36. A recent study found that SARS-CoV-2 can bind heparan sulfate on the cell surface through its spike protein. When enzymes involved in the sulfation of heparan sulfate, including NDST1, were knocked out in Hep3B cells, viral replication was almost entirely abolished12. None of these, nor the additional host factors we assessed, significantly impacted on viral replication when mutated in IOs (Fig. 5a, Fig. s9). We conclude that all of these proteins would therefore not be viable drug targets for the treatment of COVID-19 (Fig. 5b). Further studies may assess whether loss of these factors influence the cellular response to coronaviruses in any other way than replication efficiency.
TMPRSS2-dependency in SARS-CoV-2 B.1.1.7, SARS-CoV and MERS-CoV
The mutant host factor KO biobank can readily be employed when new coronaviruses or viral strains appear, to assess the dependency on host factors and identify druggable targets. We first tested whether the same TMPRSS2-dependency exists for the other two coronaviruses. SARS-CoV replication was strongly diminished upon TMPRSS2 loss, while MERS-CoV replication was reduced more modestly (Fig. 6a). The latter potential redundancy may be explained by the presence of two functional multibasic cleavage sites in the MERS-CoV spike, whereas SARS-CoV-2 and SARS-CoV possess one and none, respectively22. Both viruses could replicate in the absence of Cathepsin L, suggesting that coronaviruses generally do not use the endosomal entry route in primary epithelial cells as present in organoids (Fig. 6a).
Recently, a novel SARS-CoV-2 variant of concern (clade B.1.1.7 or Alpha) emerged and is rapidly replacing endemic viruses globally. Epidemiological data suggest that this variant is spreading 1.35–2 fold more efficiently than the ancestral lineage and is associated with higher viral loads44,45,46. Interestingly, this variant contains a mutation (P681H) directly N-terminal from the RRAR multibasic cleavage site that adds another basic residue to the multibasic cleavage site, creating an HRRAR motif. A similar mutation (P681R) was detected in the Delta variant (clade B.1.617.2). As the multibasic cleavage site facilitates serine protease-mediated entry11, mutations in or near this site may alter protease usage for S2’ cleavage, which directly triggers fusion and entry. We found that the B.1.1.7 variant replicated efficiently in wildtype and cathepsin mutant organoids, but not in TMPRSS2-deficient cells (Fig. 4e), indicating that the B.1.1.7 variant did not broaden its protease usage. These experiments provide a proof-of-concept on how emerging viral strains could be screened against mutant IOs.
The current COVID-19 pandemic has exposed weaknesses in our preparedness for coronavirus pandemics. No effective coronavirus antivirals are approved for use in humans and all completed large-scale COVID-19 drug trials have failed to show efficacy to this date, including (hydroxy)chloroquine and remdesivir8,47. The disappointing clinical effects of (hydroxy)chloroquine in humans in particular highlights gaps in the understanding of fundamental coronavirus biology. (Hydroxy)chloroquine, an inhibitor of the endosomal acidification was identified as a potent inhibitor of SARS-CoV48 and SARS-CoV-27 viral entry in cell line-based assay, confirmed here. In agreement with this, recent whole genome CRISPR/Cas9 genetic screens in transformed cell lines again suggested that endosomal entry factors, such as cathepsin L, are crucial for SARS-CoV-2 entry9,49,50.
Here, we use human intestinal organoids as a non-transformed model to study genes implicated in coronavirus biology. We have chosen to use only IOs since it is currently not possible to efficiently genetically engineer airway organoids due to limited clonal outgrowth of these cells. Nevertheless, IOs express the majority of host factors assessed, including proteases, to a similar level as the airways (Fig. 1). We confirmed that in this model ACE2 is the obligate entry receptor for SARS-CoV-2 and SARS-CoV, while DPP4 is the entry receptor for MERS-CoV, indicating that accessory receptors may not play crucial roles for these viruses. Indeed, knockout of NRP1, recently proposed as a SARS-CoV-2 (co-)receptor in Hela and Caco-2 cells, did not affect SARS-CoV-2 entry13,14. Furthermore, we demonstrate that Cathepsin L and B are not involved in SARS-CoV-2 entry in IOs. In accordance with this, a cathepsin inhibitor (E64D) and chloroquine did not inhibit SARS-CoV-2 in these IOs, while the serine protease inhibitor Camostat effectively blocked viral propagation. A similar anti-SARS-CoV-2 effect of camostat was observed in organoid-derived airway cells11. The broad activity of Camostat does not allow to pinpoint which serine protease mediates entry.
TMPRSS2-deficiency in IOs strongly decreased SARS-CoV-2 replication and spread, indicating that TMPRSS2 is the main priming protease. Other related TMPRSS genes have previously also been linked to SARS-CoV-2 replication, including TMPRSS4 in the intestine33. Overexpression of TMPRSS11D and TMPRSS13 promoted viral entry into the hamster kidney cell line BHK-2151, while TMPRSS4 overexpression facilitated viral entry in HEK293 cells33. Like TMPRSS2, TMPRSS4 is highly expressed in intestinal tissue and IOs, yet TMPRSS4 does not appear to rescue loss of TMPRSS2. This discrepancy with previous work may reflect the fact that our study relies on physiological expression of these proteases, rather than on overexpression. Importantly, intestinal organoids express similar TMPRSS family members compared to airway tissue, including high levels of TMPRSS2, TMPRSS3, TMPRSS4 and TMPRSS13. Only the TMPRSS-11A and –11D are relatively enriched in airway- versus intestinal epithelium52. Although we cannot exclude the possibility that these TMPRSS family members function in activation of SARS-CoV-2 spike in the airways, their expression levels are much lower than that of TMPRSS2 in airway organoids (Fig. 1a) and lung tissue52.
Altogether, these findings indicate that multiple TMPRSS genes may be able to mediate entry when overexpressed, but -at physiological levels in IOs- only TMPRSS2 plays an essential role, which may inspire the development of high-specificity TMPRSS2 inhibitors. The high TMPRSS-2 dependency of SARS-CoV (this study) indicates that such inhibitors may well be effective against future SARS-like coronavirus pandemics. The observation that TMPRSS2-null mice do not display a visible phenotype53 implies that such inhibitors may be well-tolerated. Our findings match with observations that SARS-CoV and to a lesser extent MERS-CoV replication and dissemination was reduced in TMPRSS2-deficient mice54.
In conclusion, our findings underscore the relevance of non-transformed human models for (corona)virus research and identify TMPRSS2 as an attractive therapeutic target in contrast to many other genes (e.g., cathepsin L, cathepsin B, NRP1, NDST1 etc.) that -as deduced from our observations- unlikely to be of clinical value. Future emerging viruses could be readily screened against our IO host factor knockout biobank to rapidly identify therapeutic targets.
Cell culture of human intestinal organoids and human airway
Human small intestinal tissue was obtained from the UMC Utrecht with informed consent of the patients. The patients wereoperated for a colorectal tumor, and a sample from non-transformed, normal mucosa was taken for this study. The study was approved by the UMC Utrecht (Utrecht, The Netherlands) ethical committee and was in accordance with the Declaration of Helsinki and according to Dutch law. This study is compliant with all relevant ethical regulations regarding research involving human participants.
Nasal inferior turbinate brushes were obtained from the Hadassah Medical Center, Jerusalem, with informed consent of the patient. Patients were diagnosed with primary ciliary dyskinesia, and tissue was obtained from healthy donors as a comparison. Healthy material was used for the RNA sequencing in this work. The study was approved by the ethical committee (Hadassah Medical Organization (HMO) IRB committee) and was in accordance with the Declaration of Helsinki and according to Israeli law under IRB approval number 075-16 HMO. This study is compliant with all relevant ethical regulations regarding research involving human participants.
Adult lung tissue was obtained from residual, tumor-free, material obtained at lung resection surgery for lung cancer. Tissue was rest material for which no informed consent was required. The Medical Ethical Committee of the Erasmus MC Rotterdam granted permission for this study (METC 2012-512).
Human small intestinal cells were isolated, processed and cultured as described previously55,56. Wnt surrogate was used (0,15 nM, U-Protein Express) instead of Wnt conditioned media. Differentiation of intestinal organoids was achieved as described previously56.
Nose tissue was dissociated and cultured as described previously57. Differentiation towards ciliated cells was performed by activating BMP signaling and inhibiting Notch signaling for 10 days (Van der Vaart et al., under review).
Isolation of human bronchial airway stem cells was performed using a protocol similar to Sachs and colleagues57. Small airway stem cells were isolated from distal human lung parenchyma as described before57. Tracheal stem cells were collected from tracheal aspirates of intubated preterm infants (28 weeks gestational age). Organoids were cultured as described before57. To obtain differentiated organoid-derived cultures, organoids were dissociated into single cells using TrypLE express (Gibco; #12604013). Cells were seeded on Transwell membranes (Corning) coated with rat tail collagen type I (Fisher Scientific). Single cells were seeded in AO growth medium: complete base medium (CBM; Stemcell Pneumacult-ALI; #05001) at a 1:1 ratio. After 2–4 days, confluent monolayers were cultured at air‐liquid interphase in CBM. Medium was changed every 5 days for 8 weeks.
Transfection of organoids for CRISPR-Cas9 experiments
sgRNAs targeting loci of interest were cloned into a SpCas9-EGFP vector (addgene plasmid #48138) using a protocol described before58. sgRNAs were designed using WTSI website (https://www.sanger.ac.uk/htgt/wge/). A full list of gRNAs and primers to generate SpCas9-EGFP expressing plasmids can be found in Supplementary Table 1. To generate homozygous frameshift mutations in genes of interest, organoids were transfected with SpCas9-EGFP containing the locus-specific sgRNA. Transient transfection using a NEPA21 electroporator was performed as described before59. 3–7 days after transfection, organoids were dissociated using TryplE (TryplE Express; Life Technologies) and sorted on a FACS-ARIA (BD Biosciences) for GFP positivity (Fig. s10) After sorting, Rho kinase inhibitor (Y-27632 dihydrochloride; 10 µM, Abmole) was added for 1 week to support single cell outgrowth.
Generation of stable genetically modified organoid lines
To generate clonal organoid lines with genotypes of preference, organoids were picked 2 weeks after sorting. Manually picked organoids were dissociated using TryplE (TryplE Express; Life Technologies) and plated in BME in pre-warmed cell culture plates. After two weeks, single cells grew into organoids and were split again to verify actively dividing stem cells. After the second split, 20 µL of organoid-BME suspension was directly taken from the plate and DNA was extracted from the organoids using the Zymogen Quick-DNA microprep kit according to protocol. Regions around sgRNA target sites were amplified using Q5 high fidelity polymerase (NEB) according to manufacturer’s protocol. CRISPR/Cas9-mediated indel formation was confirmed by sanger sequencing of these amplicons (Macrogen). Subsequently, sanger trace deconvolution was performed with the use of ICE v2 CRISPR analysis tool (synthego website) to call clonal organoid lines with homozygous frameshift mutations at the target site. Knockout clones were further expanded for viral infection experiments. Primers used for amplification and sanger sequencing can be found in Supplementary Table 1. For the generation of TMPRSS2/TMPRSS4 double mutants, TMPRSS4 was knocked out in TMPRSS2-clone 9. For the generation of CTSL/CTSB double mutants CTSL was knocked out in CTSB clone 3.
Genetically engineered organoid lines cannot be shared. Primers for the generation of these lines can be shared upon reasonable request to the corresponding authors.
Viruses and cell lines
Vero(ATCC, CCL 81) and VeroE6(ATCC, CRL 1586) cells were maintained in Dulbecco’s modified Eagle’s medium (DMEM, Gibco) supplemented with 10% fetal calf serum (FCS), HEPES, sodium bicabonate, penicillin (100 IU/mL) and streptomycin (100 IU/mL) at 37 °C in a humidified CO2 incubator. Calu-3 cells were maintained in Opti-MEM I (1X) + GlutaMAX (Gibco) supplemented with 10% FCS, penicillin (100 IU/mL) and streptomycin (100 IU/mL) at 37 °C in a humidified CO2 incubator. SARS-CoV (isolate HKU 39849, genbank accession no. AY278491), SARS-CoV-2 (isolate Bavpat-1; European Virus Archive Global #026V-03883; kindly provided by Dr. C. Drosten) were propagated on VeroE6 cells in Opti-MEM I (1X) + GlutaMAX (Gibco), supplemented with penicillin (100 IU/mL) and streptomycin (100 IU/mL) at 37 °C in a humidified CO2 incubator. MERS-CoV (isolate EMC, genbank accession no. NC019843) was propagated on Vero cells in the same medium. Non-adapted SARS-CoV-2 Bavpat-1 and B.1.1.7 (genbank accession no. MW947280) were propagated in Calu-3 cells as described before39. Stocks were produced by infecting cells at a multiplicity of infection (MOI) of 0.01 and incubating the cells for 72 h. The culture supernatant was cleared by centrifugation and stored in aliquots at −80 °C. Stock titers were determined by preparing 10-fold serial dilutions in Opti-MEM I (1X) + GlutaMAX. Aliquots of each dilution were added to monolayers of 2 × 104 VeroE6 (for SARS-CoV and SARS-CoV-2) or Vero cells (for MERS-CoV) in the same medium in a 96-well plate. Plates were incubated at 37 °C for 5 days and then examined for cytopathic effect. The TCID50 was calculated according to the method of Spearman & Kärber. All work with infectious SARS-CoV, SARS-CoV-2 and MERS-CoV was performed in a Class II Biosafety Cabinet under BSL-3 conditions at Erasmus Medical Center.
SARS-CoV, SARS-CoV-2 and MERS-CoV infection
Infections were performed using a protocol similar to17. Briefly, organoids were harvested in cold Advanced DMEM (including HEPES, Glutamax and antibiotics, termed AdDF +++17), washed once in AdDF +++, and sheared using a flamed Pasteur pipette in AdDF +++. Differentiated organoids were broken using a 5-min incubation with TrypLE (TrypLE Express; Life Technologies). After shearing, organoids were washed once in AdDF +++ before infection was performed in expansion medium. For the experiment in Fig. s5b, organoids were gently harvested using a wide pipet tip to avoid shearing organoids. A multiplicity of infection (MOI) of 0.1 was used for SARS-CoV and SARS-CoV-2 and an MOI of 0.2 was used for MERS-CoV. After 2 h of virus adsorption at 37 °C 5% CO2, cultures were washed four times with 4 ml AdDF +++ to remove unbound virus. Organoids were re-embedded into 30 μL BME in 48-well tissue culture plates and cultured in 250 μL expansion or differentiation medium at 37 °C with 5% CO2. Each well contained ~200,000 cells per well. At indicated time points cells were harvested by resuspending the BME droplet containing organoids into 200 μL AdDF +++. Samples were stored at −80 °C, a process which lysed the organoids, releasing their contents into the medium upon thawing.
For testing the antiviral activity of chloroquine diphosphate (Sigma), camostat mesylate (Sigma) and E64D (Medchemexpress) in intestinal organoids, sheared organoids were preincubated with these compounds in AdDF +++ at the indicated concentrations for 30 min at 37 °C 5% CO2 before infection at an MOI of 0.1 with SARS-CoV-2. After virus adsorption for 2 h at 37 °C 5% CO2, organoids were washed and re-embedded in BME as indicated above. Medium containing the inhibitors was added to the wells for the duration of the experiment. Cells were harvested at indicated time points as described above and stored at −80 °C.
SARS-CoV-2 entry inhibition assay by chloroquine in VeroE6 cells
Chloroquine was two-fold serially diluted in Opti-MEM I (1X) + GlutaMAX starting from a concentration of 100 µg/mL. A total of 100 μl of each dilution was added to a confluent 96-well plate of VeroE6 cells and pre-incubated at 37 °C 5% CO2 for 30 min. Next, cells were incubated with 400 plaque-forming units of virus in the same concentration range of chloroquine at 37 °C 5% CO2. After 8 h incubation, cells were fixed with formalin, permeabilized with 70% ethanol and stained with polyclonal rabbit anti-SARS-CoV nucleoprotein antibody (1:1000; 40588-T62, Sino Biological) followed by secondary Alexa488 conjugated donkey-anti-rabbit antibody (1:1000; Thermofisher Scientific, A-21206). Plates were scanned on the Amersham™ Typhoon™ Biomolecular Imager (channel Cy2; resolution 10 µm; GE Healthcare). Data was analyzed using ImageQuant TL 8.2 image analysis software (GE Healthcare).
Determination of virus titer using qRT-PCR
For determining the viral titer using qPCR, samples were thawed and centrifuged at 2000 g for 5 min. Sixty μL supernatant was lysed in 90 μL MagnaPure LC Lysis buffer (Roche) at RT for 10 min. RNA was extracted by incubating samples with 50 μL Agencourt AMPure XP beads (Beckman Coulter) for 15 min at RT, washing beads twice with 70% ethanol on a DynaMag-96 magnet (Invitrogen) and eluting in 30 μL MagnaPure LC elution buffer (Roche). Viral titers (TCID50 equivalents per mL) were determined by qRT-PCR using primer-probe sets described previously60,61,62 and comparing the Ct values to a standard curve derived from a titrated virus stock.
Immunostainings and western blot
Organoids were stained as described before55. Whole organoids were collected by gently dissolving the BME in ice-cold PBS, and subsequently fixed overnight at 4 °C in 4% paraformaldehyde (Sigma). Next, organoids were permeabilized and blocked in PBS containing 0,5% Triton X-100 (Sigma) and 2% normal donkey serum (Jackson ImunoResearch) for 30 min at room temperature. All stainings were performed in blocking buffer (2% normal donkey serum in PBS). For immunofluorescence, primary antibodies used were mouse anti-nucleoprotein (1:200; 40143-MM05, Sino Biological), mouse anti-dsRNA (1:200; Scicons, 10010200,), goat anti-ACE (1:100; R&D Systems, AF933), goat anti-DPP-4 (1:200; R&D systems, AF1180) and rabbit anti-MERS S1 (1:200; Sino Biological, 40069-T52). For immunofluorescence, organoids were incubated with the corresponding secondary antibodies; donkey anti-mouse Alexa647 (1:1000, Thermofisher Scientific, A-31571), donkey anti-rabbit Alexa488 (1:1000, Thermofisher Scientific, A-21206), donkey anti-rabbit Alexa568 (1:1000, Thermofisher Scientific, A-10042), donkey anti-goat Alexa488 (1:1000, Thermofisher Scientific, A-11055), donkey anti-goat Alexa568 (1:1000, Thermofisher Scientific, A-11057), donkey anti-goat Alexa647 (1:1000,Thermofisher Scientific, A-21447) and donkey anti-mouse Alexa568 (1:1000, Thermofisher Scientific, A-10037). or Phalloidin-Alexa488 (1:1000; Thermofisher Scientific, A12379) in blocking buffer containing 4ʹ,6-diamidino-2-phenylindole (DAPI; 1;1000; Invitrogen). After staining, organoids were transfected to a glass slide embedded in Vectashield (Vector labs). Stained organoids were imaged using a SP8 confocal microscope (Leica) or a Zeiss LSM700, and image analysis and presentation was performed using ImageJ and Leica LAS X Version 1.1 software.
Immunohistochemistry was performed as described before63. Antigen retrieval for TMPRSS2 staining was achieved by boiling for 20 min in citrate buffer. Primary antibody used was rabbit anti-TMPRSS2 (1:100; Abcam, ab109131) followed by Goat-anti-rabbit conjugated to horseradish peroxidase (1:2000, Dako, P0448) and then visualized (Powervision, Leica).
For Western blot of CTSL, organoid proteins were solubilized using a standard RIPA buffer for 30 min on ice in the presence of protease inhibitors. Samples were run on a 4–15% PAA gel (BioRad) under reducing conditions. Proteins were electrophoresed to PVDF membranes from Immobilon. Both primary antibodies, mouse anti-CTSL (±25 kDa, 1:100, Thermofisher Scientific, #BMS1032) and mouse anti-ITGB4 (±180 kDa, 1:100, Origene; AM33010PU-N), were incubated O/N at 4 C in PBS/10% milk protein/0.1% Tween20. The secondary rabbit anti-mouse HRP-conjugate (1:2000, Dako, P0260) was incubated for 2 h at 4 C in the same buffer. The mouse IgG2a antibody against ITGB4, 58XB4, was a gift from A. Sonnenberg (NKI, Amsterdam, The Netherlands). HRP activity was visualized with ECL (GE-Healthcare).
Bulk RNA sequencing
Single Cell Discoveries (Utrecht, The Netherlands) performed library preparation, using an adapted version of the CEL-seq protocol, as we have done previously17. After library generation, paired-end sequencing was performed on the Illumina Nextseq500 platform using barcoded 1 × 75 nt read setup. Read 1 was used to identify the Illumina library index and CEL-Seq sample barcode. Read 2 was aligned to the CRCh38 human RefSeq transcriptome, with the addition SARS-CoV-2 (Ref-SKU: 026V-03883) or MERS (NC_038294.1) genomes, using BWA using standard settings64. Reads that mapped equally well to multiple locations were discarded. Mapping and generation of count tables was performed using the in-house MapAndGo script, filtering to exclude reads with identical library- and molecule-barcodes. RNA sequencing data from expanding and differentiated human intestinal organoids, infected with SARS-CoV-2, was used from a previous publication17. Normalization using the median of ratios method and differential gene expression analysis was performed using the DESeq2 package64. SARS- and MERS- mapping reads were removed before normalization to avoid biasing organoid transcript counts. To generate heatmaps, row z scores of selected genes were calculated from the samples selected.
Organoid preparation for single cell sequencing analysis
Human ileal organoids were differentiated as previously described56. A control condition was kept in human organoid expansion medium to obtain stem- and progenitor cells for comparison.
Dissociation of organoids to single cells was performed by a 10-min incubation with TrypLE (TrypLE Express; Life Technologies) supported by repeated mechanical disruption using a narrowed glass pipette. Viable cells were sorted using a BD FACS Aria (BD Biosciences) using DAPI exclusion. Individual cells were collected in 384-well plates with ERCC spike-ins (Agilent), reverse transcription primers and dNTPs (both Promega). Single cell sequencing was performed according to the Sort-seq method65. Sequencing libraries were generated with TruSeq small RNA primers (Illumina) and sequenced paired-end at 60 and 26 bp read length, respectively, on the Illumina NextSeq.
Single cell RNA sequencing analysis from intestinal organoids and tissue
Reads derived from 1344 cells (192 expansion medium, 1152 differentiation medium) were mapped to the human GRCh37 genome assembly. Sort-seq read counts were filtered to exclude reads with identical library-, cell- and molecule barcodes. UMI counts were adjusted using Poisson counting statistics65. Cells with fewer than 1000 unique transcripts were excluded from further analysis. This resulted in 944 remaining cells (126 from expansion, 818 from differentiation medium)
Subsequently, RaceID3 was used for k-medoids-based clustering (knn = 5; cln = 20) of cells and differential gene expression analysis between clusters using the standard settings described at https://github.com/dgrun/RaceID3_StemID2_package. Cell types were annotated by cluster based on the expression of marker genes (OLFM4 for stem cells, FABP1 for enterocytes, FCGBP for goblet cells. Lack of these and expression of cell cycle markers including PCNA defined proliferating progenitor cells).
For comparison with tissue-derived cells, we reanalyzed a previously published dataset32 of primary human ileal cell types. To compare with the organoid data set, cells were required to be annotated as stem cell, progenitor cell, goblet cell or enterocyte and exhibit >3000 unique transcripts. This resulted in 2137 included cells, which were subsequently clustered using the standard settings of RaceID3 (cln = 16). Cells were assigned an identity based on their annotation from32.
Quantification and statistics
No statistical methods were used to predetermine sample size. The experiments were not randomized and the investigators were not blinded to the sample allocation during experiments and outcome assessment. All data are presented as mean ± standard error of the mean (SEM), unless stated otherwise. Value of n is always displayed in the figure as individual data points, and in the legends.
Statistical analysis was performed with the GraphPad Prism 9 software. We compared differences in virus replication and organoid growth by one-way ANOVA followed by a multiple-comparison test (Original FDR method of Benjamini and Hochberg; Q = 0.05) on log10 transformed values. Statistics were applied if N ≥ 3. Exact p values for all figures can be found in Supplementary dataset 5.
Further information on research design is available in the Nature Research Reporting Summary linked to this article.
The bulk and single cell RNA sequencing data generated in this study have been deposited in the Gene Expression Omnibus (GEO) database under accession codes “GSE181514” and “GSE181560”. All other relevant data supporting the key findings of this study are available within the article and its Supplementary Information files or from the corresponding author upon reasonable request. Source data are provided with this paper.
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We thank Single Cell Discoveries for RNA library preparation, and R. van der Linden and S. van Elst for help with FACS sorting. We thank E. Eenjes and R. Rottier for providing human lung material. This work was supported by: the European Research Council (Advanced Grant ERC-AdG 67013-Organoid, Cancer Research UK C6307/A29058 and The Mark Foundation for Cancer Research, the NWO building blocks of life project: Cell dynamics within lung and intestinal organoids (737.016.009), the Netherlands Organ-on-Chip Initiative, an NWO Gravitation project (024.003.001) funded by the Ministry of Education, Culture and Science of the government of the Netherlands, the NWO Gravitation project Material Driven Regeneration (024.003.013 ZWK MDR) funded by the Ministry of Education, Culture and Science of the government of the Netherlands, the Cancer Genomics Center (CGC) via the Netherlands Genomics Initiative/Netherlands Organization for Scientific research, NWO Gravitation project Material Driven Regeneration (024.003.013 ZWK MDR) funded by the Ministry of Education, Culture and Science of the government of the Netherlands, the Netherlands Organization for Health Research and Development (ZONMW) grant agreement (10150062010008 to BLH) and A donation of the Foundation Friends of the Hubrecht Institute.
H.C. is inventor on several patents related to organoid technology; his full disclosure is given at https://www.uu.nl/staff/JCClevers/. Other authors declare no competing interests.
Peer review information Nature Communications thanks the anonymous reviewer(s) for their contribution to the peer review of this work.
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Beumer, J., Geurts, M.H., Lamers, M.M. et al. A CRISPR/Cas9 genetically engineered organoid biobank reveals essential host factors for coronaviruses. Nat Commun 12, 5498 (2021). https://doi.org/10.1038/s41467-021-25729-7
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