Emergence of SARS-CoV-2 causing COVID-19 has resulted in hundreds of thousands of deaths. In search for key targets of effective therapeutics, robust animal models mimicking COVID-19 in humans are urgently needed. Here, we show that Syrian hamsters, in contrast to mice, are highly permissive to SARS-CoV-2 and develop bronchopneumonia and strong inflammatory responses in the lungs with neutrophil infiltration and edema, further confirmed as consolidations visualized by micro-CT alike in clinical practice. Moreover, we identify an exuberant innate immune response as key player in pathogenesis, in which STAT2 signaling plays a dual role, driving severe lung injury on the one hand, yet restricting systemic virus dissemination on the other. Our results reveal the importance of STAT2-dependent interferon responses in the pathogenesis and virus control during SARS-CoV-2 infection and may help rationalizing new strategies for the treatment of COVID-19 patients.
Severe acute respiratory syndrome coronavirus 2 (SARS-CoV-2) belongs to the family of Coronaviridae, which contains a large group of viruses that are constantly circulating in animals and humans. Illness in humans caused by coronaviruses is mostly mild and manifested by respiratory or digestive problems as leading symptoms1. However, some coronaviruses, such as SARS-CoV-1, Middle East respiratory syndrome-related coronavirus (MERS-CoV) and the recent SARS-CoV-2, have been responsible for serious outbreaks of severe and lethal respiratory disease2,3. Unlike the previous outbreaks with SARS-CoV-1 and MERS-CoV, the current SARS-CoV-2 outbreak has evolved as the largest global health threat to humanity in this century.
The unprecedented scale and rapidity of the current pandemic urges the development of efficient vaccines and antiviral and anti-inflammatory drugs. A key requisite in expediting this process are animal models that recapitulate and allow to understand viral pathogenesis. Such models can, hence, be used to identify new drug targets and to rationalize and preclinically assess preventive and therapeutic countermeasures.
Acute respiratory disease caused by SARS-CoV-1 and MERS infections is characterized by a dysregulated inflammatory response in which a delayed type I interferon (IFN) response promotes the accumulation of inflammatory monocyte macrophages4,5,6. The severe lung disease in coronavirus disease 2019 (COVID-19) patients seems to result from a similar overshooting inflammatory response2,7,8. However, because even non-human primates do not fully replicate COVID-199, fragmentary information and still no appropriate animal models, though urgently sought, are currently available to address this hypothesis.
In this study, we set out to understand SARS-CoV-2-induced pathogenesis by comparing SARS-CoV-2 infection in mice and hamsters, including in animals with a knockout (KO) in key components of adaptive and innate immunity. We show that mice are barely susceptible to SARS-CoV-2 infection and that viral replication in the lungs of mice is further restricted by type I IFN signaling. We demonstrate that, in contrast to mice, Syrian hamsters are highly permissive to SARS-CoV-2 infection and virus-induced lung pathology. We establish that in hamsters a dysregulated innate immune response is a driving force behind SARS-CoV-2 pathogenesis, in which in particular signal transducer and activator of transcription factor 2 (STAT2)-dependent type I and III IFN signaling plays a dual role: (i) restricting infection and dissemination on one hand but (ii) driving development of severe lung disease on the other.
Type I IFN restrict SARS-CoV-2 infection in mice
To address the lack of appropriate animal models, we first compared the effect of SARS-CoV-2 infection in wild-type (WT) mice of different lineages (BALB/c and C57BL/6) and matched transgenic mouse strains with a KO of key components of adaptive and innate immunity. We used an original patient isolate of SARS-CoV-2 (BetaCoV/Belgium/GHB-03021/2020; Supplementary Fig. 1a), passaged on HuH7 and Vero E6 cells and fully characterized by deep sequencing. No adventitious agents could be detected (Supplementary Fig. 1b, c). SARS-CoV-2 virus stocks from cell culture passage 4 (P4) and P6 were used.
To examine whether adaptive immunity contributed to the susceptibility to SARS-CoV-2 infection, we inoculated WT (immune-competent) and SCID mice (lacking functional T and B cells) from the same BALB/c background intranasally with a high 2 × 105 TCID50 (50% tissue culture infectious dose) viral dose (P4 virus) (Fig. 1a). On day 3 post inoculation (p.i.), a viral RNA peak in the lungs was observed (Fig. 1b and Supplementary Fig. 2) with no obvious differences in viral loads (Fig. 1b) or lung pathology (Fig. 1d and Supplementary Fig. 3a, b) between WT and SCID mice. These data indicate that mice that lack the human angiotensin-converting enzyme 2 (ACE2) receptor10 can in principle be infected with SARS-CoV-2, although inefficiently and likely transiently, as also observed for SARS-CoV-14,11. However, adaptive immunity did not markedly contribute to this low susceptibility.
IFNs are the prototypic first-line innate immune defense against viral infections. For many respiratory viruses, including SARS-CoV-1, in particular type I and III IFN signaling has been described to play an important role in restricting infection in vivo12. To evaluate the role of IFNs in SARS-CoV-2 infection, we compared viral RNA levels and lung pathology in WT C57BL/6 mice and C57BL/6 mice with a genetic ablation of their type I (Ifnar1−/−) and III IFN receptors (Il28r−/−) (Fig. 1a). Ifnar1−/− mice showed an enhanced replication of SARS-CoV-2 in the lung on day 3 p.i. compared to both WT and Il28r−/− mice and heat-inactivated inoculum (Fig. 1c). Similar to BALB/c mice, overall viral loads were low with some evidence for an active, although inefficient, virus replication in Ifnar1−/− mice. In general, mice of all tested strains hardly supported SARS-CoV-2 lung infection, with type I IFN signaling restricting viral replication in vivo.
WT and KO (Ifnar1−/−, Il28r−/−) mouse strains, all on C57BL/6 background, presented consistently with only a mild lung pathology. However, Ifnar1−/− mice showed increased levels of intra-alveolar hemorrhage, sometimes accompanied by some peri-bronchial inflammation (Fig. 1d and Supplementary Fig. 3a, b). Further evidence for true infection and hence viral replication was provided by transcriptomic analysis13 of infected lung tissues (Fig. 1e and Supplementary Fig. 4), revealing (i) a correlation between nucleic acid sensors TLR3/TLR9/DDX58/POLR3A and viral load (Supplementary Fig. 4, Cluster 2), (ii) an upregulation of classical antiviral effector molecules14 (enrichment P < 0.001) such as cGAS, Mx1, IFIH1/MDA-5, IRF3, OAS1, OAS3, and PKR/EIF2AK2 (Supplementary Fig. 4, Cluster 1), and (iii) downregulation of upstream regulators STAT1, STAT3, and STING/TMEM173 (Supplementary Fig. 4, Cluster 3), in agreement with a possible role for apoptosis15,16,17. In summary, our data are in line with restriction of SARS-CoV-2 infection by the IFN system in mice, as well as suggest limited inflammatory responses in the lungs of mice, in contrast to COVID-19 in humans18. Taken together, mice were considered as a poor model to study COVID-19 pathogenesis or to assess the efficacy of vaccines and treatments.
STAT2 signaling restricts SARS-CoV-2 replication in hamsters
In contrast to mice, Syrian hamsters have been reported to be highly susceptible to SARS-CoV-119 and SARS-CoV-220,21,22 infection and might thus provide a useful small animal model to study the involvement of immune responses in restricting SARS-CoV-2 infection and on SARS‑CoV-2-induced lung disease. Intranasal inoculation of SARS-CoV-2 in WT hamsters resulted indeed consistently in high viral RNA loads (Fig. 2b), a proxy used for the quantification of viral loads in the lungs (Supplementary Fig. 5), i.e., roughly 3–4 Log10 higher than in Ifnar1−/− mice (Fig. 1c), as well as high infectious titers (Fig. 2c). Pretreatment with a neutralizing SARS-CoV-1 and SARS-CoV-2-specific single-domain antibody Fc fusion construct (VHH-72-Fc)23 reduced viral loads ~105-fold in the lung of WT hamsters, further confirming an active and efficient virus replication and validating hamsters for testing of therapeutic interventions (Fig. 2f). Little, if any, viral RNA was detectable in the blood (Fig. 2d), spleen, upper small intestine, and liver of infected WT hamsters (Fig. 2e).
In order to investigate the roles of type I and III IFN during SARS-CoV-2 infection and pathogenesis, we compared virus replication levels in different tissues of WT hamsters and hamsters with ablated STAT2 (STAT2−/− lacking type I and III IFN signaling)24,25 and IL28R expression (IL28R-a−/− lacking type III IFN signaling) (Fig. 2a). Alike in WT hamsters, no signs of overt disease were recognized. Also, no marked differences were observed in viral RNA levels in the lung of WT, STAT2−/−, or IL28R-a−/− hamsters (Fig. 2b). However, in contrast to WT hamsters, STAT2−/− hamsters had significantly higher titers of infectious virus in the lung (~50-fold; Fig. 2c), along with very high levels of viral RNA detectable in blood (Fig. 2d), spleen, liver, and their upper and lower gastrointestinal tract26 (Fig. 2e). Together, these data suggest that STAT2 is critical for keeping virus replication and production of infectious progeny in the lungs down, as well as for restricting systemic SARS-CoV-2 spread and suppressing viral replication outside of the lung compartment. In line with a strong antiviral activity of STAT2 in hamsters in vivo, a similar effect was also observed in human Calu-3 cells in vitro where pharmacological inhibition of Janus-activated kinase (Jak)/STAT signaling by Ruxolitinib27,28 could fully rescue virus replication from the strong inhibitory activity of type I IFN (Fig. 2g and Supplementary Fig. 6), further underscoring the role of STAT2 in controlling virus replication, including in the human model.
STAT2 signaling drives SARS-CoV-2-induced lung disease
Next, we used these different KO hamsters to evaluate the effect of SARS-CoV-2 immune responses on lung pathology. In infected WT hamsters, a marked lung pathology characterized by an infiltration of polymorphonuclear leukocytes, bronchopneumonia, and edema was observed (Fig. 3a and Supplementary Fig. 7). This resembles histopathological findings in humans suffering from severe COVID-19 bronchopneumonia29. Inversely, the observed lung pathology was much attenuated in STAT2−/− hamsters (Fig. 3a). On the contrary, IL28R-a−/− hamsters showed clear signs of bronchopneumonia and peri-bronchiolar inflammation, similar to those observed in WT animals (Fig. 3a). In general, matching severity of lung pathology with the respective viral loads in the lungs (Fig. 3b) reveals an obvious link between infection and disease for WT and IL28R-a−/− hamsters, despite variability in individual severity scores. Much by contrast, this link is disrupted conjointly with the ablation of type I IFN responses downstream of STAT2 signaling, in face of unrestricted virus replication.
A similar picture is unveiled when assessing lung pathology by computed tomography (CT). CT imaging was established here by the lack of readily accessible serum markers and absence of overt disease symptoms as a non-invasive means to score for SARS-CoV-2-induced lung disease, alike in standard patient care to aid COVID-19 diagnosis with high sensitivity and monitor progression/recovery7,8,30,31. Similar as in humans32, semi-quantitative lung pathology scores were obtained from high-resolution chest micro-CT scans of free-breathing animals33. Pulmonary consolidations were present in SARS-CoV-2-infected WT and IL28R-a−/− hamsters but not in STAT2−/− hamsters (Fig. 3c and Supplementary Fig. 8). Apart from lung consolidations and airway dilation as main observed pathology, marked differences in other micro-CT-derived markers of specific lung pathology, such as hyperinflation, emphysema, or atelectasis34,35, were not observed, except in one animal that presented with hyperinflation (Supplementary Fig. 8c). Again, STAT2−/− hamsters showed minimal lung involvement (Fig. 3c). Further quantitative analysis34 revealed an increase of the non-aerated lung volume in SARS-CoV-2-infected WT and IL28R-a−/− hamsters, yet again not in STAT2−/− hamsters (Fig. 3d and Supplementary Fig. 8e). First, these data fully support micro-CT as a convenient adjunct to histological scoring (Fig. 3d, e and Supplementary Fig. 8a–e) to visualize and quantify SARS-CoV-2-induced lung injury in the hamster model. Moreover, it may allow to monitor the impact of therapeutic measures non-invasively during disease progression. Second, of relevance for COVID-19 immunopathogenesis, virus replication was unlinked from lung disease in STAT2−/− hamsters (Supplementary Fig. 8f).
An elevation of serum levels of several cytokines such as interleukin (IL)-6, IL-10, and IFN-γ is reported in critically ill COVID-19 patients2,7,8. Intriguingly, these genes were also induced in the lungs of infected hamsters (Fig. 3f, g and Supplementary Fig. 9a), along with elevated mRNA levels of IP-10 (CXCL-10) as reported for other cytokines/chemokines downstream of IFN-γ20, and of MX-2 downstream of type I and III IFNs. However, WT, STAT2−/−, and IL28R-a−/− hamsters each showed marked differences in the respective expression levels (Fig. 3f), with overall strongest induction in WT hamsters. First of all, IFN-stimulated genes36 such as MX-2 (strongly induced by type I IFN/STAT2 signaling) and IP-10 (induced by both type I and type II IFNs) showed a differential expression pattern when comparing the different genotypes, triggered by SARS-CoV-2 infection. Lower baseline expression of MX-2 and IP-10 and failure to respond to SARS-CoV-2 infection by MX-2 upregulation in STAT2−/− hamsters confirmed the functional KO (Supplementary Fig. 9a). As expected, IL28R-a−/− hamsters showed an intermediate phenotype between that of WT and STAT2−/− concerning their antiviral IFN response. Of note, the receptor KOs did not affect ACE2 expression37,38 in the hamster lungs (Supplementary Fig. 9a). Importantly, the expression levels of IP-10 and MX-2, and to a lesser extent also of IL-6 (Fig. 3g, h; for other possible molecular markers, see Supplementary Fig. 9b), correlated with the disease severities observed in the respective hamster strains (Fig. 3a, c–e), with lowest inflammatory and antiviral cytokine responses in the absence of STAT2-dependent type I and III IFN signaling.
For the development of efficient therapeutic interventions against SARS-CoV-2, relevant small animal models are needed that mimic the different clinical manifestations of COVID-19 and that provide fundamental mechanistic insight into the underlying pathology/pathogenesis. Transgenic mice expressing hACE2, the bona fide receptor of SARS-CoV-1 and SARS-CoV-239, have been suggested as COVID-19 model40,41,42. We here demonstrate that WT mice are also susceptible to SARS-CoV-2 infection, yet resulting in very limited viral replication and inflammatory responses. Ablation of type I IFN signaling in Ifnar1−/− mice results in the same small incremental 10-fold increase in viral replication as was originally reported for SARS-CoV-139,43 in hACE2 transgenic mice, though recent data suggest an approximate 100-fold increase for SARS-CoV-2 in such models40,42. Nevertheless, neither mouse model fully recapitulates pathogenesis of COVID-19 nor allows the study of clinical SARS-CoV-2 isolates without prior adaptation44. It remains of interest to investigate the added effect of both (i) hACE2 knock-in, and (ii) Ifnar and/or Il28r KO in mice12,45. In fact, in WT mice that had been transduced using adenoviral vectors expressing hACE2 to facilitate SARS-CoV-2 infection, concomitant blockage of IFNAR by receptor-neutralizing antibodies resulted in enhanced disease46.
In contrast to mice, SARS-CoV-2 infection and associated pathology in WT hamsters seems to resemble what has been reported for SARS-CoV-1 in the same model, confirmed in the meantime also by others20,21,22. An early peak of active virus replication was noted in the lungs with viremia and extra-pulmonary spread. This was accompanied by a strong acute inflammatory response19 (as visualized by histopathology) with induction of IL-6, IL-10, and IFN-γ expression (albeit with some variation between animals) like in humans2,7,8,47,48 and, as a consequence, pulmonary damage that could readily be depicted as tissue consolidations and obstruction of the lungs by chest micro-CT as established in this study. Micro-CT may hence become a key instrument to non-invasively and quantitatively monitor SARS-CoV-2 lung disease. This will allow to conveniently monitor the effect of therapeutic strategies and test the preclinical efficacy of vaccine candidates.
In humans, SARS-CoV-2 infection begins frequently with a flu-like illness, followed in a second phase by an intense inflammatory response characterized by a cytokine storm and acute lung injury (ALI) and respiratory distress syndrome (ARDS) associated with high mortality2,7,8. Considering the very acute and short-lived infection kinetics observed in intranasally inoculated hamsters20,21 that may not allow for full development of protracted (bi-phasic) COVID-19-like disease22, we studied SARS-CoV-2-induced pathology as early as 4 days p.i. Nevertheless, main pathological findings seem to resemble to a large extent what is observed in humans. Some variability in infection outcome, in particular in pathology scores of WT hamsters (Fig. 3b, h and Supplementary Fig. 8f), may be explained by two experimental constraints. First, the genetics of WT hamsters that are outbred and may hence show a varying susceptibility, as hypothesized in humans27. Second, the use of SARS-CoV-2 stocks from two passages P4 and P6 virus stocks. Sequencing analysis of the virus stocks revealed two small in-frame deletions in Spike (S) glycoprotein (i.e., in the N-terminal domain and the furin-cleavage site49,50,51; Supplementary Fig. 1b, c) to dominate in the P6 virus used, likely as a consequence of adaptation to enhanced growth in Vero E6 cells in vitro. This observation is in line with earlier reports, namely, of tissue culture-adaptive mutations similar to those observed by us (Supplementary Fig. 1b, c) resulting in reduced fitness of SARS-CoV-2 in WT hamsters (no body weight loss and attenuation of pathology)52, emphasizing possible consequences of using cell culture-adapted virus when studying SARS-CoV-2 infection in animal models.
By using unique KO hamster lines, we demonstrated that STAT2 plays a critical role in mediating antiviral responses and restricting systemic dissemination of SARS-CoV-2 (see Fig. 3i for a summary of phenotypes). This is in line with the effect of STAT1 in a mouse model of SARS-CoV-1 infection53. However and much in contrast to what is generally observed for viral infections in Stat2−/− mice54 or STAT2−/− hamsters25,55,56, the severe pathology induced by SARS-CoV-2 in WT hamsters is not observed in the absence of STAT2. Indeed, pneumonia as assessed by sensitive micro-CT was absent in STAT2−/− hamsters. Considering the established negative regulation of IL-6 and other mediators of inflammation by STAT254,57, our hamster model may help to understand the immune pathogenesis of ALI and ARDS caused by highly pathogenic coronaviruses12,19,58 as well as other respiratory viruses4. Of note, a meta-analysis of infected human cells revealed a specific SARS-CoV-2-regulated transcriptional footprint for STAT2 in particular that was stronger than that of any other inflammatory transcription factor59.
The increase in replication of SARS-CoV-2 seen in IL28R-a−/− hamsters, on one hand, combined with a tempered inflammatory response and lung injury as compared to WT hamsters, on the other hand, is in line with the role type III IFN plays during respiratory virus infections, including in SARS-CoV-145. This observation also suggests that in humans pegylated IFN-lambda60,61 (or similar modulators of innate immunity) may possibly be considered to protect medical staff and other frontline workers from SARS-CoV-2 infection or to dampen symptoms in critically ill patients62, however, with caution considering a potential pathophysiological role of IFN-lambda63,64.
In conclusion, hamsters may be preferred above mice as infection model for the preclinical assessment of antiviral therapies, of vaccines, and of approaches that aim at tempering the COVID-19 immune pathogenesis in critically ill patients18,65. The latter may be achieved by repurposing anti-inflammatory drugs66 such as IL-6 receptor antagonists (e.g., Tocilizumab)67,68,69,70 or small molecule Jak/STAT inhibitors (e.g., Ruxolitinib71,72 or Tofacitinib). Educated by our finding that STAT2 signaling plays a dual role in also limiting viral dissemination, targeting the virus-induced cytokine response and overshooting of macrophage activation may need to be complemented by (directly acting) antivirals73.
WT Syrian hamsters (Mesocricetus auratus) were purchased from Janvier Laboratories. All other mouse (C57BL/6, Ifnar1−/−, Il28r−/−, BALB/c, and SCID) and hamster (STAT2−/− and IL28R-a−/−) strains were bred in-house. Six-to-8-week-old female mice and female WT hamsters were used throughout the study. KO hamsters were used upon availability: 7–12-week-old female STAT2−/− hamsters and 5–7-week-old IL28R-a−/− hamsters.
Ifnar1−/− mouse breeding couples were a generous gift of Dr. Claude Libert, IRC/VIB, University of Ghent, Belgium. Il28r−/− mice [C57B/6N-A<tm1Brd>Ifnlr1<tm1a(EUCOMM)Wtsi>/Wtsi, strain ID: EM:07988] were provided by the Wellcome Trust Sanger Institute Mouse Genetics Project (Sanger MGP)74.
STAT2−/− and IL28R-a−/− hamsters were generated by CRISPR/Cas-mediated gene targeting. To ablate STAT2 (Gene ID: 101830537) expression, a 1-nt frameshift mutation was introduced in exon 4 resulting in multiple premature stop codons24; to ablate IL28R (IFNLR1; Gene ID: 101833778) expression, a 22-nucleotide deletion was introduced in exon 2 resulting in multiple premature stop codons in the original open reading frame.
Animals were housed individually (hamsters) or per 5 (mice) in individually ventilated isolator cages (IsoCage N Biocontainment System, Tecniplast) at a temperature of 21 °C, humidity of 55%, and 12:12 dark/light cycles, with access to food and water ad libitum, and cage enrichment (cotton and cardboard play tunnels for mice, wood block for hamsters). Housing conditions and experimental procedures were approved by the ethical committee of KU Leuven (license P015-2020), following institutional guidelines approved by the Federation of European Laboratory Animal Science Associations (FELASA). Animals were euthanized by 100 µl (mice) or 500 µl (hamsters) of intraperitoneally (i.p.) administered Dolethal (200 mg/ml sodium pentobarbital, Vétoquinol SA). Animals were monitored daily for signs of disease (lethargy, heavy breathing, or ruffled fur).
Prior to infection, the animals were anesthetized by i.p. injection of a xylazine (16 mg/kg, XYL-M®, V.M.D.), ketamine (40 mg/kg, Nimatek, EuroVet), and atropine (0.2 mg/kg, Sterop) solution. Each animal was inoculated intranasally by gently adding 50 µl droplets of virus stock containing 2 × 105 TCID50 (P4 virus) or 2 × 106 TCID50 (P6 virus) in both nostrils. Uninfected animals did not receive any virus or matrix. Due to time constraints by the pandemic outbreak and the urgency to develop a small animal model, we have used virus stock from two different passages (P4 and P6) to characterize our model. A full genotypic characterization of the viruses used is provided in Supplementary Fig. 1, and phenotypic differences and virus titers are provided in the text and legends.
Cells, virus, and sera
Vero E6 (African green monkey kidney, kind gift from Peter Bredenbeek, LUMC, NL) and HuH7 (human hepatoma, JCRB0403) cells were maintained in minimal essential medium (Gibco) supplemented with 10% fetal bovine serum (Integro), 1% bicarbonate (Gibco), and 1% L-glutamine (Gibco). For maintenance of Calu-3 cells (human airway epithelium, kind gift from Lieve Naesens, KU Leuven, BE), the above medium was supplemented with 10 mM HEPES (Gibco). All assays involving virus growth were performed using 2% (Vero E6 and HuH7) or 0.2% (Calu-3) fetal bovine serum instead of 10%.
SARS-CoV-2 strain BetaCov/Belgium/GHB-03021/2020 (EPI ISL 407976|2020-02-03) recovered from a nasopharyngeal swab taken from a reverse transcription quantitative polymerase chain reaction (RT-qPCR)-confirmed asymptomatic patient returning from Wuhan, China beginning of February 202075 was directly sequenced on a MinION platform (Oxford Nanopore)76. Phylogenetic analysis confirmed a close relation with the prototypic Wuhan-Hu-1 2019-nCoV (GenBank accession number MN908947.3) strain. Infectious virus was isolated by serial passaging on HuH7 and Vero E6 cells (see Supplementary Fig. 1), with the addition of penicillin/streptomycin, gentamicin, and amphotericin B. Virus used for animal experiments was from passages P4 and P6. Prior to inoculation of animals, virus stocks were confirmed to be free of mycoplasma (PlasmoTest, InvivoGen) and other adventitious agents by deep sequencing on a MiSeq platform (Illumina) following an established metagenomics pipeline77,78. The infectious content of virus stocks was determined by titration on Vero E6 cells by the Spearman–Kärber method. All virus-related work was conducted in the high-containment BSL3+ facilities of the KU Leuven Rega Institute (3CAPS) under licenses AMV 30112018 SBB 219 2018 0892 and AMV 23102017 SBB 219 2017 0589 according to institutional guidelines.
Antibody VHH-72-Fc was administered i.p. at a dose of 20 mg/kg 1 day prior to infection. VHH-72-Fc was expressed in ExpiCHO cells (ThermoFisher Scientific) and purified from the culture medium as described23. Briefly, after transfection with pcDNA3.3-VHH-72-Fc plasmid DNA, followed by incubation at 32 °C and 5% CO2 for 6–7 days, the VHH-72-Fc protein in the cleared cell culture medium was captured on a 5 ml MabSelect SuRe column (GE Healthcare), eluted with a McIlvaine buffer pH 3, neutralized using a saturated Na3PO4 buffer, and buffer exchanged to storage buffer (25 mM L-Histidine, 125 mM NaCl). The antibody’s identity was verified by protein- and peptide-level mass spectrometry.
RNA extraction and RT-qPCR
Animals were euthanized at different time points postinfection, organs were removed, and lungs were homogenized manually using a pestle and a 12-fold excess of cell culture medium (Dulbecco’s modified Eagle’s medium/2% fetal calf serum). RNA extraction was performed from homogenate of 30 mg of lung tissue with the RNeasy Mini Kit (Qiagen), or 50 µl of serum using the NucleoSpin Kit (Macherey-Nagel), according to the manufacturer’s instructions. Other organs were collected in RNALater (Qiagen) and homogenized in a bead mill (Precellys) prior to extraction. Of 100 µl eluate, 4 µl was used as template in RT-qPCR reactions. RT-qPCR was performed on a LightCycler96 platform (Roche) using the iTaq Universal Probes One-Step RT-qPCR Kit (BioRad) with primers and probes (Supplementary Table 1) specific for SARS-CoV-2, mouse β-actin (Actb), and hamster β-actin (ACTB), IL6, IL10, IFNλ, IFNγ, MX2, IP-10, TNFα, and ACE2 (IDT). SARS-CoV-2 qPCR reactions were carried out in duplicate for each data point. Standards of SARS-CoV-2 cDNA (IDT) and infectious virus were used to express the amount of RNA as normalized viral genome equivalent copies per milligram tissue or as TCID50 equivalents per milliliter serum, respectively. The mean of housekeeping gene β-actin was used for normalization. The relative fold change was calculated using the 2−ΔΔCt method79.
Quantification of SARS-CoV-2 infectious particles in lung tissues
After extensive transcardial perfusion with phosphate-buffered saline (PBS), lungs were collected, extensively homogenized using manual disruption (Precellys24) in minimal essential medium (5% w/v), and centrifuged (12,000 rpm, 10 min, 4 °C) to pellet the cell debris. Infectious SARS-CoV-2 particles were quantified by means of endpoint titrations on confluent Vero E6 cell cultures. Viral titers were calculated by the Spearman–Kärber method and expressed as the TCID50 per 100 mg tissue.
Differential gene expression and bioinformatics analysis
To study differential gene expression, RNA was extracted from lung tissues using Trizol, subjected to cDNA synthesis (High Capacity cDNA Reverse Transcription Kit, Thermo Fisher Scientific) and qPCR using a custom Taqman qRT-PCR array (Thermo Fisher Scientific) of 30 genes known to be activated in response to virus infection13, as well as two housekeeping genes (Supplementary Table 2). Data collected were analyzed using the Quant Studio Design and Analysis (version 1.5.1) and Data Assist software (version 3.01, Thermo Fisher Scientific). Pathway, Gene Ontology, and transcription factor target enrichment analysis was performed using Gene Set Enrichment Analysis (Molecular Signatures Database (MSigDB), Broad Institute). Principal component analysis, correlation matrices, and unsupervised hierarchical clustering (Euclidean distance) were performed using XLSTAT and visualized using MORPHEUS (https://software.broadinstitute.org/morpheus)17.
For histological examination, the lungs were fixed overnight in 4% formaldehyde and embedded in paraffin. Tissue sections (4 µm) were stained with hematoxylin and eosin to visualize and score for lung damage.
In vitro JAK/STAT inhibition assay
Calu-3 (human airway epithelial) cells were plated at 5 × 104 cells/well in a 96-well plate and incubated overnight with 4 µM of the JAK1/2 inhibitor Ruxolitinib80 (Toronto Research Chemicals, ON, Canada). Next day, cells were pretreated for 4 h with 10 IU/ml of Universal type I IFN (PBL Assay Science, NJ, USA, cat. no. 11200) before infection with SARS-CoV-2 (P4 or P6, 5 × 103 TCID50 per well). Two hours post infection, cells were washed with PBS and incubated for an additional 48 h with IFN and Ruxolitinib before collection of the supernatant for RNA extraction and quantification of virus yields by RT-qPCR.
Micro-CT and image analysis
Hamsters were anesthetized using isoflurane (Iso-Vet) (2–3% in oxygen) and installed in prone position into the X-cube micro-CT scanner (Molecubes) using a dedicated imaging bed. Respiration was monitored throughout. A scout view was acquired and the lung was selected for a non-gated, helical CT acquisition using the High-Resolution CT protocol, with the following parameters: 50 kVp, 960 exposures, 32 ms/projection, 350 µA tube current, rotation time 120 s. Data were reconstructed using a regularized statistical (iterative) image reconstruction algorithm using non-negative least squares81, using an isotropic 100 µm voxel size, and scaled to Hounsfield Units after calibration against a standard air/water phantom. The spatial resolution of the reconstruction was estimated at 200 µm by minimizing the mean squared error between the three-dimensional reconstruction of the densest rod in a micro-CT multiple density rod phantom (Smart Scientific) summed in the axial direction and a digital phantom consisting of a two-dimensional disk of 17.5 mm radius that was post-smoothed with Gaussian kernels using different full width half maxima, after aligning the symmetry axis of the rod to the z-axis.
Visualization and quantification of reconstructed micro-CT data was performed with DataViewer and CTan software (Bruker micro-CT). As primary outcome parameter, a semi-quantitative scoring of micro-CT data was performed33,34,82 with minor modifications toward optimization for COVID-19 lung disease in hamsters. In brief, visual observations were scored (from 0 to 2 depending on severity, both for parenchymal and airway disease) on 5 different, predefined transversal tomographic sections throughout the entire lung image for both lung and airway disease by two independent observers (L.S. and G.V.V.) and averaged. Scores for the 5 sections were summed up to obtain a score from 0 to 10 reflecting severity of lung and airway abnormalities compared to scans of healthy, WT control hamsters. As secondary measures, image-derived biomarkers (non-aerated lung volume, aerated lung volume, total lung volume, the respective densities within these volumes, and large airway volume) were quantified as in refs. 33,82 for a manually delineated volume of interest in the lung, avoiding the heart and main blood vessels. The threshold used to separate the airways and aerated (gray value 0–55) from non-aerated lung volume (gray value 56–255) was set manually on an 8-bit grayscale histogram and kept constant for all data sets.
GraphPad Prism Version 8 (GraphPad Software, Inc.) was used for all statistical evaluations. The number of animals and independent experiments that were performed is indicated in the legends to figures. Statistical significance was determined using non-parametric Mann–Whitney U test for pairwise comparisons or Kruskal–Wallis test with Dunn’s post hoc test for multiple comparisons. Values were considered significantly different at P values of ≤0.05.
Further information on research design is available in the Nature Research Reporting Summary linked to this article.
SARS-CoV-2 strain BetaCov/Belgium/GHB-03021/2020 sequence is available from GISAID (EPI ISL 407976|2020-02-03, https://www.gisaid.org). Prototypic Wuhan-Hu-1 2019-nCoV sequence is available from GenBank (accession number MN908947.3). All data supporting the findings in this study are also available from the corresponding author upon request. Source data are provided with this paper.
Cui, J., Li, F. & Shi, Z. L. Origin and evolution of pathogenic coronaviruses. Nat. Rev. Microbiol. 17, 181–192 (2019).
Zhu, N. et al. A novel coronavirus from patients with pneumonia in China, 2019. N. Engl. J. Med. 382, 727–733 (2020).
Chen, J. et al. Clinical progression of patients with COVID-19 in Shanghai, China. J. Infect. 80, e1 (2020).
Channappanavar, R. et al. Dysregulated type I interferon and inflammatory monocyte-macrophage responses cause lethal pneumonia in SARS-CoV-infected mice. Cell Host Microbe 19, 181–193 (2016).
Channappanavar, R. & Perlman, S. Pathogenic human coronavirus infections: causes and consequences of cytokine storm and immunopathology. Semin. Immunopathol. 39, 529–539 (2017).
Page, C. et al. Induction of alternatively activated macrophages enhances pathogenesis during severe acute respiratory syndrome coronavirus infection. J. Virol. 86, 13334–13349 (2012).
Wang, D. et al. Clinical characteristics of 138 hospitalized patients with 2019 novel coronavirus-infected pneumonia in Wuhan, China. JAMA 323, 1061–1069 (2020).
Huang, C. et al. Clinical features of patients infected with 2019 novel coronavirus in Wuhan, China. Lancet 395, 497–506 (2020).
Rockx, B. et al. Comparative pathogenesis of COVID-19, MERS, and SARS in a nonhuman primate model. Science 368, 1012–1015 (2020).
Hoffmann, M. et al. SARS-CoV-2 cell entry depends on ACE2 and TMPRSS2 and is blocked by a clinically proven protease inhibitor. Cell 181, 271.e8–280.e8 (2020).
Ishii, K. et al. Neutralizing antibody against severe acute respiratory syndrome (SARS)-coronavirus spike is highly effective for the protection of mice in the murine SARS model. Microbiol. Immunol. 53, 75–82 (2009).
Mahlakõiv, T. et al. Combined action of type I and type III interferon restricts initial replication of severe acute respiratory syndrome coronavirus in the lung but fails to inhibit systemic virus spread. J. Gen. Virol. 93, 2601–2605 (2012).
Sharma, S. et al. Small molecule inhibitors of TBK1 serve as adjuvant for a plasmid-launched live-attenuated yellow fever vaccine. Hum. Vaccines Immunother. 16, 2196–2203 (2020).
Schoggins, J. W. Interferon-stimulated genes: what do they all do? Annu. Rev. Virol. 6, 567–584 (2019).
Khouri, R. et al. A genetic IFN/STAT1/FAS axis determines CD4 T stem cell memory levels and apoptosis in healthy controls and Adult T-cell Leukemia patients. Oncoimmunology 7, e1426423 (2018).
Van Weyenbergh, J., Wietzerbin, J., Rouillard, D., Barral-Netto, M. & Liblau, R. Treatment of multiple sclerosis patients with interferon-beta primes monocyte-derived macrophages for apoptotic cell death. J. Leukoc. Biol. 70, 745–748 (2001).
Delgobo, M. et al. An evolutionary recent IFN/IL-6/CEBP axis is linked to monocyte expansion and tuberculosis severity in humans. Elife 8, e47013 (2019).
Zumla, A., Hui, D. S., Azhar, E. I., Memish, Z. A. & Maeurer, M. Reducing mortality from 2019-nCoV: host-directed therapies should be an option. Lancet 395, e35–e36 (2020).
Roberts, A. et al. Severe acute respiratory syndrome coronavirus infection of golden Syrian hamsters. J. Virol. 79, 503–511 (2005).
Chan, J. F.-W. et al. Simulation of the clinical and pathological manifestations of Coronavirus Disease 2019 (COVID-19) in golden Syrian hamster model: implications for disease pathogenesis and transmissibility. Clin. Infect. Dis. https://doi.org/10.1093/cid/ciaa325 (2020).
Sia, S. F. et al. Pathogenesis and transmission of SARS-CoV-2 in golden hamsters. Nature 583, 834–838 (2020).
Imai, M. et al. Syrian hamsters as a small animal model for SARS-CoV-2 infection and countermeasure development. Proc. Natl Acad. Sci. USA 117, 16587–16595 (2020).
Wrapp, D. et al. Structural basis for potent neutralization of betacoronaviruses by single-domain camelid antibodies. Cell 181, 1436–1441 (2020).
Fan, Z. et al. Efficient gene targeting in golden Syrian hamsters by the CRISPR/Cas9 system. PLoS ONE 9, e109755 (2014).
Toth, K. et al. STAT2 knockout Syrian hamsters support enhanced replication and pathogenicity of human adenovirus, revealing an important role of type I interferon response in viral control. PLoS Pathog. 11, e1005084 (2015).
Lin, L. et al. Gastrointestinal symptoms of 95 cases with SARS-CoV-2 infection. Gut 69, 997–1001 (2020).
Bagca, B. G. & Avci, C. B. The potential of JAK/STAT pathway inhibition by ruxolitinib in the treatment of COVID-19. Cytokine Growth Factor Rev. 54, 51–61 (2020).
Felgenhauer, U. et al. Inhibition of SARS-CoV-2 by type I and type III interferons. J. Biol. Chem. 295, 13958–13964 (2020).
Xu, Z. et al. Pathological findings of COVID-19 associated with acute respiratory distress syndrome. Lancet Respir. Med. 8, 420–422 (2020).
Ai, T. et al. Correlation of chest CT and RT-PCR testing in coronavirus disease 2019 (COVID-19) in China: a report of 1014 cases. Radiology 296, E32–E40 (2020).
Chen, T. et al. Clinical characteristics of 113 deceased patients with coronavirus disease 2019: retrospective study. BMJ 368, m1091 (2020).
Shi, H. et al. Radiological findings from 81 patients with COVID-19 pneumonia in Wuhan, China: a descriptive study. Lancet Infect. Dis. 20, 425–434 (2020).
Poelmans, J. et al. Longitudinal, in vivo assessment of invasive pulmonary aspergillosis in mice by computed tomography and magnetic resonance imaging. Lab. Investig. 96, 692–704 (2016).
Vande Velde, G. et al. Longitudinal micro-CT provides biomarkers of lung disease that can be used to assess the effect of therapy in preclinical mouse models, and reveal compensatory changes in lung volume. DMM Dis. Model. Mech. 9, 91–98 (2016).
de Langhe, E. et al. Quantification of lung fibrosis and emphysema in mice using automated micro-computed tomography. PLoS ONE 7, e43123 (2012).
Zivcec, M., Safronetz, D., Haddock, E., Feldmann, H. & Ebihara, H. Validation of assays to monitor immune responses in the Syrian golden hamster (Mesocricetus auratus). J. Immunol. Methods 368, 24–35 (2011).
Ziegler, C. G. K. et al. SARS-CoV-2 receptor ACE2 is an interferon-stimulated gene in human airway epithelial cells and is detected in specific cell subsets across tissues. Cell 181, 1016.e19–1035.e19 (2020).
Onabajo, O. O. et al. Interferons and viruses induce a novel primate-specific isoform dACE2 and not the SARS-CoV-2 receptor ACE2. Preprint at https://doi.org/10.1101/2020.07.19.210955 (2020).
Mccray, P. B. et al. Lethal infection of K18-hACE2 mice infected with severe acute respiratory syndrome coronavirus. J. Virol. 81, 813–821 (2007).
Jiang, R. Di et al. Pathogenesis of SARS-CoV-2 in transgenic mice expressing human angiotensin-converting enzyme 2. Cell 182, 50.e8–58.e8 (2020).
Bao, L. et al. The pathogenicity of SARS-CoV-2 in hACE2 transgenic mice. Nature 583, 830–833 (2020).
Sun, S. H. et al. A mouse model of SARS-CoV-2 infection and pathogenesis. Cell Host Microbe 28, 124.e34–133.e4 (2020).
Yang, X. H. et al. Mice transgenic for human angiotensin-converting enzyme 2 provide a model for SARS coronavirus infection. Comp. Med. 57, 450–459 (2007).
Gu, H. et al. Adaptation of SARS-CoV-2 in BALB/c mice for testing vaccine efficacy. Science 369, 1603–1607 (2020).
Mordstein, M. et al. Lambda interferon renders epithelial cells of the respiratory and gastrointestinal tracts resistant to viral infections. J. Virol. 84, 5670–5677 (2010).
Hassan, A. O. et al. A SARS-CoV-2 infection model in mice demonstrates protection by neutralizing antibodies. Cell 182, 744.e4–753.e4 (2020).
Tay, M. Z., Poh, C. M., Rénia, L., MacAry, P. A. & Ng, L. F. P. The trinity of COVID-19: immunity, inflammation and intervention. Nat. Rev. Immunol. 20, 363–374 (2020).
Liu, J. et al. Longitudinal characteristics of lymphocyte responses and cytokine profiles in the peripheral blood of SARS-CoV-2 infected patients. EBioMedicine 55, 102763 (2020).
Andersen, K. G., Rambaut, A., Lipkin, W. I., Holmes, E. C. & Garry, R. F. The proximal origin of SARS-CoV-2. Nat. Med. 26, 450–452 (2020).
Zhang, T., Wu, Q. & Zhang, Z. Probable pangolin origin of SARS-CoV-2 associated with the COVID-19 outbreak. Curr. Biol. 30, 1346.e2–1351.e2 (2020).
Wrapp, D. et al. Cryo-EM structure of the 2019-nCoV spike in the prefusion conformation. Science 367, 1260–1263 (2020).
Lau, S.-Y. et al. Attenuated SARS-CoV-2 variants with deletions at the S1/S2 junction. Emerg. Microbes Infect. 9, 837–842 (2020).
Frieman, M. B. et al. SARS-CoV pathogenesis is regulated by a STAT1 dependent but a type I, II and III interferon receptor independent mechanism. PLoS Pathog. 6, 1–14 (2010).
Park, C., Li, S., Cha, E. & Schindler, C. Immune response in Stat2 knockout mice. Immunity 13, 795–804 (2000).
Gowen, B. B. et al. Modeling severe fever with thrombocytopenia syndrome virus infection in golden Syrian hamsters: importance of STAT2 in preventing disease and effective treatment with favipiravir. J. Virol. 91, e01942-16 (2017).
Siddharthan, V. et al. Zika virus infection of adult and fetal STAT2 knock-out hamsters. Virology 507, 89–95 (2017).
Gough, D. J., Messina, N. L., Clarke, C. J. P., Johnstone, R. W. & Levy, D. E. Constitutive type I interferon modulates homeostatic balance through tonic signaling. Immunity 36, 166–174 (2012).
Liu, L. et al. Anti-spike IgG causes severe acute lung injury by skewing macrophage responses during acute SARS-CoV infection. JCI Insight 4, e123158 (2019).
Ochsner, S. A., Pillich, R. T. & McKenna, N. J. Consensus transcriptional regulatory networks of coronavirus-infected human cells. Sci. Data 7, 314 (2020).
Yurdaydin, C. New treatment options for delta virus: is a cure in sight? J. Viral Hepat. 26, 618–626 (2019).
Andreakos, E., Zanoni, I. & Galani, I. E. Lambda interferons come to light: dual function cytokines mediating antiviral immunity and damage control. Curr. Opin. Immunol. 56, 67–75 (2019).
Prokunina-Olsson, L. et al. COVID-19 and emerging viral infections: the case for interferon lambda. J. Exp. Med. 217, e20200653 (2020).
Major, J. et al. Type I and III interferons disrupt lung epithelial repair during recovery from viral infection. Science 369, eabc2061 (2020).
Broggi, A. et al. Type III interferons disrupt the lung epithelial barrier upon viral recognition. Science 369, eabc3545 (2020).
Liu, Q., Zhou, Y. H. & Yang, Z. Q. The cytokine storm of severe influenza and development of immunomodulatory therapy. Cell. Mol. Immunol. 13, 3–10 (2016).
Cully, M. Immune status could determine efficacy of COVID-19 therapies. Nat. Rev. Drug Discov. 19, 431–434 (2020).
Kang, S., Tanaka, T., Narazaki, M. & Kishimoto, T. Targeting interleukin-6 signaling in clinic. Immunity 50, 1007–1023 (2019).
Portsmore, S., Tran Nguyen, T. N., Beacham, E. & Neelakantan, P. Combined IL-6 and JAK/STAT inhibition therapy in COVID-19-related sHLH, potential game changer. Br. J. Haematol. https://doi.org/10.1111/bjh.16966 (2020).
Jordan, S. C. et al. Compassionate use of tocilizumab for treatment of SARS-CoV-2 pneumonia. Clin. Infect. Dis. https://doi.org/10.1093/cid/ciaa812 (2020).
Morillas, J. A. et al. Tocilizumab therapy in five solid and composite tissue transplant recipients with early ARDS due to SARS-CoV-2. Am. J. Transplant. https://doi.org/10.1111/ajt.16080 (2020).
Foss, F. M. et al. Attenuated novel SARS coronavirus 2 infection in an allogeneic hematopoietic stem cell transplant patient on ruxolitinib. Clin. Lymphoma Myeloma Leuk. 20, 720–723 (2020).
Koschmieder, S. et al. Favorable COVID-19 course despite significant comorbidities in a ruxolitinib-treated patient with primary myelofibrosis. Eur. J. Haematol. 105, 655–658 (2020).
Agostini, M. L. et al. Coronavirus susceptibility to the antiviral remdesivir (GS-5734) is mediated by the viral polymerase and the proofreading exoribonuclease. MBio 9, e00221-18 (2018).
White, J. K. et al. XGenome-wide generation and systematic phenotyping of knockout mice reveals new roles for many genes. Cell 154, 452 (2013).
Spiteri, G. et al. First cases of coronavirus disease 2019 (COVID-19) in the WHO European Region, 24 January to 21 February 2020. Euro Surveill. 25, 2000178 (2020).
Vrancken, B. et al. Accounting for population structure reveals ambiguity in the Zaire Ebolavirus reservoir dynamics. PLoS Negl. Trop. Dis. 14, e0008117 (2020).
Conceição-Neto, N. et al. Modular approach to customise sample preparation procedures for viral metagenomics: a reproducible protocol for virome analysis. Sci. Rep. 5, 16532–16532 (2015).
Conceição-Neto, N., Yinda, K. C., Van Ranst, M. & Matthijnssens, J. NetoVIR: modular approach to customize sample preparation procedures for viral metagenomics. Methods Mol. Biol. 1838, 85–95 (2018).
Livak, K. J. & Schmittgen, T. D. Analysis of relative gene expression data using real-time quantitative PCR and the 2−ΔΔCT method. Methods 25, 402–408 (2001).
Stewart, C. E., Rall, R. E. & Adamson, C. S. Inhibitors of the interferon response enhance virus replication in vitro. PLoS ONE 9, e112014 (2014).
Vandeghinste, B. et al. Iterative CT reconstruction using shearlet-based regularization. IEEE Trans. Nucl. Sci. 60, 3305–3317 (2013).
Berghen, N. et al. Radiosafe micro-computed tomography for longitudinal evaluation of murine disease models. Sci. Rep. 9, 17598 (2019).
We thank Kathleen Van den Eynde, Eef Allegaert, Sarah Cumps, Wilfried Versin, Caroline Collard, Elke Maas, Jasper Rymenants, Jasmine Paulissen, Nathalie Thys, Céline Sablon, Catherina Coun, and Madina Rasulova for excellent technical assistance. We thank Johan Nuyts for support with imaging file processing; Pieter Mollet for support with the micro-CT installation; Jef Arnout and Annelies Sterckx and Animalia and Biosafety Departments of KU Leuven for facilitating the studies. We also thank Dr. Claude Libert for providing the Ifnar1−/− mice and the Wellcome Trust Sanger MGP for providing the Il28r−/− mutant mouse line. This project has received funding from the European Union’s Horizon 2020 research and innovation program (No. 101003627 and No. 733176), funding from BMGF (INV-00636), FWO Flanders (VirEOS project 30981113), the FWO Hercules Foundation, the KU Leuven Rega Foundation, “Internal Funds KU Leuven” awarded to P.M. (project 3M170314), and the Stichting Antoine Faes. J.Ma was supported by the China Scholarship Council (CSC), J.M.-C. by a doctoral grant from HONOURs Marie-Sklodowska-Curie training network (721367), B.V. by a FWO Flanders SB grant (1S28617N), C.C. by the FWO (1001719N), G.V.V. by KU Leuven Internal Funds (C24/17/061), K.D. by KU Leuven Internal Funds (C3/19/057 Lab of Excellence), G.O. and E.M. by KU Leuven Internal Funds (C16/17/010) and by FWO Flanders, D.D.V. by an FWO SB grant, and B.S. by FWO-EOS project VIREOS. COVID-19 research in the X.S. and N.C. laboratories is supported by VIB, by a Ghent University GOA grant, and VIB, UGent and FWO emergency Covid-19 grants.
D.D.V., B.S., and X.S. are named as inventors on US patent application no. 62/988,610, entitled “Coronavirus Binders.” D.D.V., B.S., X.S., and N.C. are named as inventors on US patent application no. 62/991,408, entitled “SARS-CoV-2 Virus Binders.”
Peer review information Nature Communications thanks the anonymous reviewers for their contribution to the peer review of this work.
Publisher’s note Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
About this article
Cite this article
Boudewijns, R., Thibaut, H.J., Kaptein, S.J.F. et al. STAT2 signaling restricts viral dissemination but drives severe pneumonia in SARS-CoV-2 infected hamsters. Nat Commun 11, 5838 (2020). https://doi.org/10.1038/s41467-020-19684-y
The importance of routine quality control for reproducible pulmonary measurements by in vivo micro-CT
Scientific Reports (2022)
The oral protease inhibitor (PF-07321332) protects Syrian hamsters against infection with SARS-CoV-2 variants of concern
Nature Communications (2022)
Nature Communications (2022)
Patient-derived monoclonal antibody neutralizes SARS-CoV-2 Omicron variants and confers full protection in monkeys
Nature Microbiology (2022)
Molecular Imaging and Biology (2022)