Deficiency in coatomer complex I causes aberrant activation of STING signalling

Steiner, Annemarie; Hrovat-Schaale, Katja; Prigione, Ignazia; Yu, Chien-Hsiung; Laohamonthonkul, Pawat; Harapas, Cassandra R.; Low, Ronnie Ren Jie; De Nardo, Dominic; Dagley, Laura F.; Mlodzianoski, Michael J.; Rogers, Kelly L.; Zillinger, Thomas; Hartmann, Gunther; Gantier, Michael P.; Gattorno, Marco; Geyer, Matthias; Volpi, Stefano; Davidson, Sophia; Masters, Seth L.

doi:10.1038/s41467-022-29946-6

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Published: 28 April 2022

Deficiency in coatomer complex I causes aberrant activation of STING signalling

Nature Communications volume 13, Article number: 2321 (2022) Cite this article

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Abstract

Coatomer complex I (COPI) mediates retrograde vesicular trafficking from Golgi to the endoplasmic reticulum (ER) and within Golgi compartments. Deficiency in subunit alpha causes COPA syndrome and is associated with type I IFN signalling, although the upstream innate immune sensor involved was unknown. Using in vitro models we find aberrant activation of the STING pathway due to deficient retrograde but probably not intra-Golgi transport. Further we find the upstream cytosolic DNA sensor cGAS as essentially required to drive type I IFN signalling. Genetic deletion of COPI subunits COPG1 or COPD similarly induces type I IFN activation in vitro, which suggests that inflammatory diseases associated with mutations in other COPI subunit genes may exist. Finally, we demonstrate that inflammation in COPA syndrome patient peripheral blood mononuclear cells and COPI-deficient cell lines is ameliorated by treatment with the small molecule STING inhibitor H-151, suggesting targeted inhibition of the cGAS/STING pathway as a promising therapeutic approach.

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Introduction

COPA syndrome is a recently identified rare disorder, involving complex pathology with dysregulation of the innate and adaptive immune system¹. The disease is caused by autosomal dominant mutations in the COPA gene, which encodes the α−subunit (COPα, COPA) of the coatomer complex I (COPI). COPI mediates retrograde trafficking of cargo proteins from Golgi to the endoplasmic reticulum (ER) and within cis-Golgi compartments². To date, more than 17 families with mutations in COPA have been identified worldwide^3,4. Clinically, symptoms occur with varying severity, including interstitial lung disease with or without pulmonary haemorrhage, inflammatory arthritis, immune-mediated kidney disease and autoantibodies, which develop in the majority of patients¹.

Disease onset occurs during childhood or early adulthood with incomplete penetrance, leaving some individuals unaffected, despite carrying the mutation¹. Interestingly, across all reported COPA syndrome patients, a total of 11 missense mutations have been identified, almost all located within exon 8 and 9 of the COPA gene, which translates into a 14 amino acid stretch (aa.230-243) within the WD40 domain of the COPA protein^3,4. Being highly conserved between species and implicated in protein-protein interactions, COPA mutants were shown to have impaired binding efficiency to dilysine-motif-containing cargo proteins, therefore causing defective retrograde transport¹. As a consequence, ER stress, activation of the unfolded protein response (UPR) and nuclear factor kappa B (NF-κB) pathway activation were suggested pathomechanisms, which have already been linked to lung disease and autoimmunity in other studies⁵.

Furthermore, Volpi and colleagues were the first to describe elevated transcription levels of type I interferons (IFNs) and interferon-stimulated genes (ISGs) in peripheral blood of COPA syndrome patients, suggesting a role of type I IFN signalling and a dysregulated innate immune response in disease pathogenesis⁶. This finding is supported by three recent case reports showing the therapeutic benefit of Janus kinase (JAK) 1/2 inhibition in COPA syndrome patients^7,8,9. However, the innate immune sensor, as well as the molecular mechanisms underlying COPA syndrome pathogenesis remained unclear.

Due to the involvement of COPA in intracellular trafficking, and its subcellular localization, we hypothesised COPA could play a possible role in STING (stimulator of IFN gene, also known as MITA, MPYS and ERIS)^10,11,12,13 pathway regulation. Inactive STING forms homodimers that localize to the ER membrane and has been identified as a signalling molecule downstream of multiple intracellular nucleotide sensors including cyclic GMP-AMP synthase (cGAS)^14,15. cGAS recognizes cytosolic double-stranded DNA independent of its sequence as a danger-associated molecular pattern (DAMP) and synthesises 2’3’-cGAMP, a second messenger detected by STING¹⁶. 2’3’-cGAMP binding results in a conformational change in STING, which enables translocation to the Golgi apparatus¹⁷. Downstream signalling occurs via IκB kinase epsilon (IKKε)- and TANK-binding-kinase 1 (TBK1)-mediated activation of transcription factors NF-κB and IFN regulatory factor 3 (IRF3)¹⁸. Translocation of these transcription factors to the nucleus then results in gene expression of proinflammatory cytokines and type I and III IFNs (IFNαβ and IFNλ)^19,20.

Identifying the innate immune pathway activated in COPA syndrome will provide valuable insights in disease pathology leading to beneficial pharmacological intervention for this inflammatory condition.

Results

Generation of cellular models for COPA syndrome

Aiming to study the protein function of COPA in the context of innate immune signalling, we used CRISPR/Cas9 genome editing to delete COPA in human monocytic THP-1 and epithelial HeLa cell lines. This approach was based on the assumption that the reduced target protein binding efficiency of loss of function mutations identified in COPA syndrome patients can be mimicked by the reduction of wild-type (WT) COPA protein levels. Using single guide (sg) RNAs targeting different exons of the COPA gene under a Doxycycline (Dox)-inducible promoter, we generated three COPA-deficient THP-1 cells lines. Interestingly, the reduction of COPA protein levels coincided with spontaneous phosphorylation of the transcription factor signal transducer and activator of transcription 1 (STAT1), which is downstream of type I and III IFN signalling (Fig. 1a)^21,22. Using this experimental approach, complete deletion of COPA could not be achieved long-term because COPA is essential for cell survival²³. To circumvent this, we performed Dox-induced COPA deletion prior to every experiment and proceeded to use the THP-1 cell line with sgRNA 1 (subsequently termed COPA^deficient) as it demonstrated the greatest reduction in COPA levels and concomitantly increased STAT1 phosphorylation (pSTAT1) (Fig. 1a).

**Fig. 1: Cell line models for COPA syndrome.**

Elevated proinflammatory cytokine gene expression levels (IL1B, IL6, IL12, IL4, IL23) have previously been described in B cell lines derived from COPA syndrome patients and a type I IFN gene signature was reported in patient peripheral blood mononuclear cells (PBMCs)^1,6. Similarly, qRT-PCR analysis of our COPA^deficient THP-1 cells revealed increased mRNA expression levels of proinflammatory cytokines (TNF and IL6), the type I IFN subtypes IFNA1 and IFNB1 as well as ISGs, such as ISG15, IFIT1 and MX1 (Fig. 1b). Furthermore, increased protein levels of IFNβ and the IFN-induced chemokine, CXCL10 ^24,25 were measured by ELISA in supernatants from COPA^deficient THP-1 cells (Fig. 1c).

In order to independently confirm these findings in a different cell line, we used the same experimental approach and sgRNA1 to delete COPA in epithelial HeLa cells (Fig. 1d). Similar to THP-1 cells, the reduction of COPA protein levels in HeLa cells resulted in increased transcription of proinflammatory cytokines and type I IFN-induced genes (Fig. 1e), as well as elevated baseline phosphorylation of TBK1 (pTBK1), a signalling molecule downstream of several pattern recognition receptors (Fig. 1d)^19,26. Although silencing of the cGAS/STING pathway due to immortalisation with viral oncogenes in HeLa cells has been reported²⁷, we confirmed pathway activity in this particular cell line used here by stimulation with synthetic DNA analogues (Supplementary Fig. 1). Therefore, we have successfully generated COPA^deficient THP-1 and HeLa cell lines that model inflammatory manifestations observed in COPA syndrome and present a useful tool to investigate the molecular mechanisms underlying this disease.

Inflammatory signalling in COPA syndrome model cell lines is driven by STING pathway overactivation

To identify the innate immune sensor that is driving the inflammatory response in our in vitro model of COPA syndrome, we genetically co-deleted several candidate innate immune receptors in COPA^deficient THP-1 cells (Supplementary Fig. 2). Using a hypothesis-driven approach, we excluded the involvement of inflammasome sensor NLRP3 (Supplementary Fig. 2a), cytoplasmic RNA sensor protein kinase R (PKR) (Supplementary Fig. 2b) and RNA-sensors retinoic acid-inducible gene-I (RIG-I) and melanoma differentiation-associated protein 5 (MDA5) by deletion of the shared adaptor protein mitochondrial antiviral-signalling protein (MAVS) (Supplementary Fig. 2c). Furthermore, deletion of Unc93 homolog B1 (UNC93B1), an adaptor protein essential for stability and signalling of endosomal Toll-like receptors (TLRs) and cell surface TLR5²⁸, was not able to ameliorate the inflammatory phenotype in COPA^deficient THP-1 cells (Supplementary Fig. 2d).

Another candidate immune sensor is STING, which triggers inflammation downstream of multiple cytoplasmic nucleic acid sensors including cGAS^16,29,30. Inactive STING localizes on the ER membrane and requires coatomer complex II (COPII)-mediated anterograde trafficking to translocate to Golgi compartments upon activation^{31,32,33,34,35}. Although COPA is not a part of the COPII complex, all compartments of the secretory pathway form a tightly regulated and interdependent network within the cell³⁶. Therefore, we hypothesized that reduced functionality of COPA-mediated retrograde transport might potentially interfere with STING trafficking and cause aberrant signalling. In line with this, we identified COPA as a potential interaction partner for STING in an unbiased mass spectrometry-based quantitative proteomics experiment, where we analysed protein lysates from HEK293T cells following the pulldown of overexpressed mCitrine (mCit)-tagged human STING (Fig. 2a, Supplementary Data 1). Furthermore, this screen identified SURF4 as a potential STING-interactor, which was recently shown to act as adapter protein mediating STING-COPA interaction for subsequent retrograde trafficking^37,38. Additionally, other known STING-interacting proteins were found to be enriched in STING pulldowns, including TBK1. Although not significantly enriched, other COPI/COPII subunit proteins and ER- and Golgi-resident proteins were identified, highlighting the importance of the secretory pathway for STING regulation (Supplementary Data 1). Interestingly, transmembrane protein 214 (TMEM214), involved in ER stress-induced caspase-4 activation and induction of apoptosis³⁹, was highly enriched in STING pulldowns; however, a functional link to STING has not yet been described in the literature and was not further investigated in this study.

**Fig. 2: Inflammation induced by COPA-deficiency is STING dependent.**

CRISPR/Cas9-mediated genetic co-deletion of STING ameliorated the spontaneous pSTAT1 signal (Fig. 2b) as well as inflammatory gene expression in COPA^deficient THP-1 cells (Fig. 2c). Interestingly, TNF transcription levels remained high after STING deletion and are likely the result of NF-κB pathway activation following ER stress, as previously suggested¹. We independently confirmed this result by genetic deletion of STING in COPA^deficient HeLa cells, which ameliorated type I IFN-mediated inflammatory baseline signalling and the pTBK1 signal (Supplementary Fig. 3). Furthermore, in the context of potential pharmaceutical intervention, treatment of COPA^deficient THP-1 cells with small-molecule STING inhibitor H-151 was able to markedly reduce baseline STAT1 phosphorylation (Fig. 2d) and type I IFN-mediated gene transcription (Fig. 2e), thus indicating a possible targeted treatment for COPA syndrome patients.

ER-to-Golgi translocation of STING is a prerequisite for interaction with downstream signalling molecules^10,17,40. We therefore aimed to investigate the cellular localization of STING in COPA-deficiency and performed immunofluorescence (IF) staining of endogenous STING in HeLa cells (Fig. 2f). As positive control, parental HeLa cells were stimulated with HT-DNA, a double-stranded DNA molecule to activate cGAS-induced STING ER-to-Golgi translocation which can be observed as distinct puncta formation (Fig. 2f). However, in COPA^deficient HeLa cells without further stimulation, puncta formation of endogenous STING was not as clear and rather suggested the formation of multiple smaller size specks distributed throughout the cytoplasm (Fig. 2f). Since the overall signal of stained endogenous STING was quite weak, we stably overexpressed STING-GFP in these cell lines via retroviral transduction. Parental cells showed the diffuse cytoplasmic distribution of STING-GFP when untreated and the formation of puncta that co-localized with cis-Golgi marker GM130 following HT-DNA transfection (Supplementary Fig. 4a, b). In COPA-deficient cells, multiple STING-GFP speckles were observed, which largely co-localized with cis-Golgi marker (GM130) (Supplementary Fig. 4a, b). Co-localization with ER marker KDEL was not different when compared to parental cells (Supplementary Fig. 4c). Considering that loss of COPA is associated with Golgi dispersal⁴¹ (Supplementary Fig. 4, 5) and spontaneously accumulated STING-GFP co-localized with Golgi but not ER markers, these experiments suggest that STING signalling occurs due to spontaneous accumulation at the dispersed Golgi in this in vitro model of COPA syndrome.

Overall, these results suggest that spontaneous STING activation is driving the inflammatory response in COPA syndrome model THP-1 and HeLa cell lines, which is likely the result of STING accumulation at dispersed Golgi fragments.

Mutations in COPA drive STING-dependent inflammation

In order to validate our findings in patient samples, we analysed PBMCs from a COPA syndrome patient carrying the c.698 G > A (R233H) mutation with clinical presentation of severe polyarticular arthritis and lung disease⁶. At the time of sample collection, the patient was treated with prednisone and rituximab. Ex vivo flow cytometry analysis revealed elevated levels of pTBK1, particularly in CD14-expressing monocytes (Supplementary Fig. 6). Treatment with STING inhibitor H-151 was able to ameliorate baseline TBK1 phosphorylation as shown in representative histograms and quantified as fold change of pTBK1 levels after H-151 treatment (measured by geometric mean fluorescence intensity (MFI)), thereby confirming basal STING activation in patient PBMCs (Fig. 3a, b).

**Fig. 3: Mutations in COPA trigger STING-dependent inflammation.**

To further study inflammation in the context of COPA syndrome, we generated overexpression plasmids encoding the previously published loss of function COPA mutations E241K and R233H¹. Initially, we overexpressed these constructs in HEK293T cells which lack detectable levels of endogenous STING^16,42 (Supplementary Fig. 7). Phosphorylation of TBK1 and IRF3 was only observed when myc-tagged COPA was co-expressed with mCit-tagged STING (Fig. 3c). However, in this system, STING is transiently overexpressed at high levels. This results in strong baseline activation of WT STING alone, observed by above background pTBK1 and pIRF3 signal (Fig. 3c), likely caused by spontaneous dimerization-induced Golgi translocation and subsequent pathway activation⁴³, which is a commonly observed disadvantage of this experimental setup. STING signalling was slightly elevated by co-expression with WT COPA. Rather than a specific effect of WT COPA, this observation is likely the result of high-level protein translation following co-transfection that overwhelms ER folding and retrograde transport capacities and subsequently causes STING retention at the Golgi that promotes signalling. Interestingly, when co-expressed with COPA mutants STING activation was markedly increased, which suggests that impaired retrograde trafficking prevents Golgi-to-ER retrieval and promotes STING accumulation at Golgi compartments, which results in increased signalling (Fig. 3c).

Therefore, we sought to test a more physiological setting with lower, stable expression of STING-GFP incorporated via lentiviral transduction of HEK293T cells and subsequent FACS sorting for low expression close to endogenous level. Surprisingly, under these conditions, the overexpression of COPA mutants E241K and R233H was not able to drive inflammation (Fig. 3d). In order to independently confirm this finding, we transiently transfected COPA E241K and R233H using 2 different plasmid concentrations in HEK293 cells, which express endogenous STING at levels comparable to HeLa cells (Supplementary Fig. 7). Again, in this system, overexpression of COPA mutants was not able to induce pIRF3 over empty vector (EV) control levels (Fig. 3e).

Importantly, these experiments suggest that inflammation driven by COPA mutations in HEK239T cells only occurs when STING is overexpressed. However, with endogenous levels of STING expression, as in HEK293 cells or HEK293T cells stably expressing STING-GFP, overexpressed COPA mutations cannot drive inflammation, likely because an essential player of the COPA syndrome pathology is lacking in these cell lines. Given that all the downstream machinery required for STING signalling appears to be intact in HEK293T cells (Fig. 3c) we wondered if the missing part of the pathway was actually upstream, specifically the cytoplasmic DNA sensor cGAS, since it is not endogenously expressed in HEK293(T) cells (Supplementary Fig. 7).

Inflammatory signalling in COPA^deficient THP-1 cells is cGAS-dependent

In order to investigate the involvement of cGAS in COPA syndrome pathology, CRISPR/Cas9 gene editing was employed to delete COPA in a monoclonal cGAS knockout (cGAS^−/−) THP-1 cell line⁴⁴. Lack of cGAS completely abolished spontaneous phosphorylation of STAT1, which was re-established upon reconstitution with GFP-tagged cGAS⁴⁵ via lentiviral transduction (Fig. 4a). Similarly, transcription levels of proinflammatory cytokines and ISGs were ameliorated in COPA^deficient cells when cGAS was deleted (Fig. 4b). Interestingly, co-deleted COPA^deficient/cGAS^−/− THP-1 cells showed stronger reduction in TNF gene transcription compared to STING deletion in COPA^deficient THP-1 cells (Fig. 2c). One reason for this could be that the cGAS^−/− cells are monoclonal and completely lack cGAS expression⁴⁴, whereas the STING^−/− cells are a mixed population of CRISPR/Cas9-deleted cells, with some residual STING expression. However, clonal cGAS deletion was still not able to fully reverse TNF transcription to baseline levels, which supports the involvement of ER stress as additional NF-κB activating pathway¹.

**Fig. 4: Inflammatory signalling in COPA^deficient THP-1 cells requires cGAS.**

Recently, the role of SURF4 as an adapter protein that mediates packaging of STING into COPI vesicles was established^37,38. In support of this, our mass spectrometry analysis identified SURF4 as an interactor of STING after overexpression in HEK293T cells (Fig. 2a). Assuming that lack of SURF4 specifically blocks Golgi-to-ER trafficking of STING and other SURF4 target proteins, we found increased phosphorylation of STAT1 and elevated transcription of ISGs following the genetic deletion of SURF4 in THP-1 WT cells (Supplementary Fig. 8; preliminary data). This phenotype was ablated in cGAS^−/−/SURF4^−/− THP-1 cells (Supplementary Fig. 8, preliminary data) further supporting the requirement of cGAS as the initial driver for STING accumulation at the Golgi and subsequent inflammatory signalling in COPA syndrome.

To further confirm cGAS activation, we analysed cytoplasmic levels of cGAS-produced second messenger 2’3’-cGAMP by ELISA. Surprisingly, 2’3’-cGAMP levels in COPA^deficient THP-1 cells were significantly elevated over parental controls (Fig. 4c). This result suggests cGAS activation above tonic levels in COPA-deficiency, however, whether this is the primary defect driving COPA syndrome pathology remains to be validated in COPA mutant-expressing cells.

We then sought to investigate cGAS/STING pathway activity upon cGAS stimulation with foreign DNA (HT-DNA and poly (dA:dT)) and analysed cytoplasmic 2’3’-cGAMP production. Surprisingly, after stimulation, lower 2’3’-cGAMP levels were detected in cells lacking COPA, suggesting reduced cGAS activation following targeted stimulation (Fig. 4d). In order to independently confirm this result, three different COPA-deficient THP-1 cells lines (from Fig. 1a) were stimulated with HT-DNA, poly (dA:dT) and small-molecule STING activator 2’3’-c-di-AM(PS)₂ (abbreviated: c-di-AM(PS)₂). Cellular supernatants were collected and analysed for levels of IFNλ, a type III IFN which is similarly activated to type I IFN upon PRR stimulation^46,47 (Fig. 4e). In line with the previous result, all tested COPA-deficient cell lines were less responsive to cGAS stimulation when compared to parental control cells. Yet interestingly, direct STING stimulation by the cGAMP analogue was not impaired and comparable across all cell lines (Fig. 4e).

Together, this data demonstrates that cGAS is required for inflammation driven by COPA-deficiency in THP-1 cells, and that the second messenger 2’3’-cGAMP is elevated in these cells, indicating increased cGAS activity. However, despite this increased activation, it is no longer possible to activate cGAS with transfected cytoplasmic DNA, indicating that this is a breakpoint in the pathway that is impacted in COPA syndrome.

Spontaneous cGAS/STING signalling is activated by general deficiency in COPI-mediated retrograde transport

Besides COPA (subunit α), 6 other subunit proteins COPB1 (β), COPB2 (β’), COPD (δ), COPE (ε), COPG (γ), COPΖ (ξ) as well as the small GTPase ARF1 are essential for functional retrograde trafficking between Golgi and ER and within cis-Golgi compartments (Fig. 5a)². Here, we sought to determine whether activation of the cGAS/STING signalling pathway is uniquely linked to loss of COPA function, or whether disruption of the retrograde trafficking route in general results in inflammation via this pathway. Therefore, we randomly selected COPI-subunits COPG1, COPD and COPE and used the CRISPR/Cas9 technology to delete these subunits in HeLa and THP-1 cells.

**Fig. 5: cGAS/STING pathway activation is caused by general deficiency in COPI-mediated retrograde trafficking.**

To confirm that retrograde transport is indeed impaired upon silencing of the selected COPI subunits, we used immunofluorescence super-resolution microscopy and investigated the localization and intensity of KDEL staining in COPI subunit-deficient HeLa cells (Fig. 5b). The amino acid sequence KDEL is an ER-specific retention signal encoded on the C-terminus of soluble ER-resident proteins that undergo Golgi-to-ER retrieval through COPI-mediated retrograde transport⁴⁸. We therefore hypothesized that impaired retrograde transport would result in the accumulation of KDEL signal within Golgi compartments. Overall, COPI-deficient cells showed increased KDEL signal intensity compared to parental controls (Fig. 5b), which is likely the consequence of increased expression of KDEL-tagged ER chaperones following ER stress and UPR activation^1,49,50. Indeed, when compared to parental cells with intact retrograde transport, a significant shift in KDEL localization towards Golgi compartments was observed in COPA^deficient, COPG1^deficient and COPD^deficient HeLa cells (Fig. 5b). Quantification of this result is shown as the area ratio of KDEL signal overlaying with cis-Golgi marker GM130 divided by total area of KDEL staining per cell (Fig. 5c). These results indicate that genetic deletion of COPA, COPG1 or COPD results in impaired retrograde trafficking, which is similar to the functional defect described for COPA mutants¹. Immunoblotting confirmed that unless intentionally deleted, only minor variability is observed for COPA, COPG1 and COPD protein expression levels across COPI subunit-deficient THP-1 cell lines (Fig. 5d). Therefore, despite deletion of selected subunits, expression levels of tested residual COPI proteins remain largely stable suggesting that destabilization or complete co-depletion of subunits does not occur. As one exception, COPE expression levels are markedly reduced in COPA^deficient cells (Fig. 5d). In yeast, COPE was shown to be non-essential for functional retrograde transport, but its role as a structural component to stabilize COPA at higher temperatures has been described⁵¹. Since COPE expression levels are dependent on COPA binding and coatomer integration⁵², co-depletion of both proteins in COPA^deficient cells is not surprising, however, this was not observed when COPE was intentionally deleted. This indicates that COPE is not required for COPA stability and functional retrograde transport in human cells under the culture conditions used here. In line with this, only deficiency in COPI complex proteins COPA, COPG1 and COPD but not COPE resulted in spontaneous inflammatory signalling (Fig. 5d,e). In order to determine whether the inflammatory phenotype can be ameliorated by inhibition of cGAS/STING signalling, COPI subunit-deficient THP-1 cells were treated with STING inhibitor H-151. Immunoblot as well as qRT-PCR analysis showed reduction of STAT1 phosphorylation (Fig. 5d) and decreased transcription of proinflammatory genes and ISGs after inhibitor treatment (Fig. 5e). These data demonstrate that indeed, the cGAS/STING pathway is activated upon deletion of different COPI subunit proteins, and therefore a general defect in retrograde transport sufficiently induces inflammatory signalling. Consequently, aberrant STING signalling is unlikely to be the unique result of reduced COPA function.

Also similar to the loss of COPA, COPG1-deficiency results in a break in cGAS signalling upon stimulation with HT-DNA and poly (dA:dT), but IFNλ release following STING stimulation with c-di-AM(PS)₂ remains comparable to control cells or higher (Supplementary Fig. 9), further highlighting the essential role of intact retrograde transport for functional cellular defence in response to foreign DNA.

Retrograde trafficking between Golgi and ER is the transport direction underlying STING mislocalization in COPI-deficiency

Besides Golgi-to-ER retrieval of proteins, the COPI complex is also required for trafficking within Golgi compartments⁵³. Disruption of which of these transport directions causes defective STING regulation in COPA syndrome has not yet been experimentally examined.

Within the cells, trafficking of cargo proteins via different COPI transport routes is thought to be regulated through multiple COPI complex isotypes⁵⁴, consisting of different combinations of subunits γ and ζ paralogues termed γ1 (COPG1), γ2 (COPG2), ζ1 (COPZ1), ζ2 (COPZ2)^55,56. Localization studies revealed spatial segregation of COPG paralogues, with COPG1 and COPG2 being predominantly enriched in cis-Golgi or trans-Golgi compartments, respectively⁵⁷, which was suggested to reflect functional heterogeneity and specific roles. Based on cellular localization, COPG1 was suggested to be more likely involved in mediating retrograde transport between Golgi and ER while COPG2 is thought to serve the intra-Golgi transport route⁵⁷. Taking advantage of this proposed functional distinction, we deleted COPG1 and COPG2 isoforms individually in THP-1 WT cells using the CRISPR/Cas9 approach. Deletion efficiency was confirmed by immunoblotting for COPG1 and COPG2 transcript analysis by qRT-PCR due to the lack of a specific antibody (Fig. 6a, b). Interestingly, only deletion of COPG1 resulted in spontaneous phosphorylation of STAT1 and inflammatory gene transcription, whereas this was not observed in COPG2^deficient cells (Fig. 6a, c). Amelioration of inflammatory signalling in COPG1^deficient cells was achieved by treatment with STING inhibitor H-151 (Fig. 5d, e), indicating STING pathway activation in COPG1^deficient THP-1 cells due to defective retrograde transport, whereas deletion of COPG2, implicated in intra-Golgi transport, had no effect.

**Fig. 6: Targeted inhibition of anterograde intra-Golgi transport does not activate spontaneous STING signalling.**

Despite the described differences in localization of COPG1- and COPG2-containing COPI vesicles within secretory pathway compartments⁵⁷, the suggested functional difference between both paralogues has not yet been confirmed experimentally⁵⁸. Proteomic profiling of γ1ζ1, γ1ζ2, γ2ζ1−COPI vesicle contents did not reveal significant differences⁵⁹, however, mediation of specific transport directions has not been investigated.

Therefore, in an alternative approach, we specifically blocked intra-Golgi trafficking by pharmacological inhibition of the cytosolic Ca²⁺-dependent phospholipase A₂ alpha (cPLA2α)⁶⁰, which is required for the formation of intercisternal tubules that connect Golgi stacks and are essential for intra-Golgi transport^60,61. Treatment of immortalized bone marrow-derived macrophages (iBMDMs) with cPLA2α inhibitor arachidonyl trifluoromethyl ketone (AACOCF3) did not result in spontaneous phosphorylation of TBK1, indicating that defective intra-Golgi trafficking does not sufficiently activate spontaneous STING signalling (Fig. 6d). Since cPLA2α was shown to be involved in regulating inducible nitric oxide synthase (iNOS) expression⁶², we confirmed AACOCF3 activity by evaluating expression levels of iNOS in response to IFNγ and lipopolysaccharide (LPS) stimulation. Pretreatment with cPLA2α inhibitor reduced iNOS levels (Fig. 6d), thereby validating inhibitor functionality at the used concentrations⁶³, although off-target effects cannot be ruled out.

COPI-mediated formation of early endosome has been shown to be required for autophagy⁴¹. Importantly, functional autophagy and lysosomal degradation pathways are required for the termination of STING signalling^34,64,65. Therefore, a possible defect in those pathways caused by COPA deficiency was excluded by monitoring STING expression levels during Dox-induced COPA depletion (96 hours (hrs) Dox treatment) in THP-1 cells (Supplementary Fig. 10). Progressive loss of COPA did not coincide with the accumulation of STING, suggesting the normal function of STING degradation pathways.

Together these findings indicate, that although COPA as part of the COPI complex mediates multiple transport directions within the secretory pathway, the disease-causing mechanism in COPA deficiency relies on defective retrograde trafficking, specifically lost Golgi-to-ER retrieval of immune signalling protein STING.

Collectively, our results demonstrate that aberrant STING signalling in cell lines lacking COPA is the result of defective retrograde trafficking which impairs steady-state Golgi-to-ER retrieval of STING and causes subsequent accumulation at Golgi compartments. Spontaneous inflammation was dependent on upstream dsDNA detector cGAS in THP-1 cell lines, which suggests the requirement of a STING-activating stimulus to induce pathogenicity. However interestingly, cGAS no longer responded sufficiently to cytoplasmic DNA stimulation suggesting a break in the cGAS/STING signalling axis due to COPA deficiency. The finding that deletion of other COPI subunits, such as COPG1 or COPD, impart a similar cellular phenotype suggests that immune-mediated disorders associated with mutations in other COPI subunit proteins may exist.

Discussion

In this study, we have generated model cell lines that recapitulate the type I IFN signature observed in PBMCs of COPA syndrome patients⁶. We show that the type I IFN signature can be ablated by genetic deletion and pharmacological inhibition of STING and also its upstream regulator cGAS, a cytosolic DNA sensor. Interestingly, the clinical phenotype of COPA syndrome partially overlaps with symptoms reported in STING-associated vasculopathy with onset in infancy (SAVI), including severe systemic inflammation, recurrent fevers, interstitial lung disease, early onset in life and a predominant constitutive type I IFN gene activation^66,67. For SAVI, multiple case reports identified gain of function mutations in STING, causing spontaneous dimerization, Golgi translocation and STING pathway activation⁶⁸. Localization studies of endogenous STING and reconstituted STING-GFP in COPA^deficient HeLa cells showed STING accumulation in multiple small specks scattered throughout the cytosol, which partially co-localized with dispersed Golgi fragments in preliminary experiments. Partial Golgi dispersal and redistribution has previously been observed in COPA-deficient cell lines⁴¹ and also occurs after secretory pathway inhibition by treatment with Brefeldin-A, a small GTPase inhibitor that prevents initiation of COPI and II vesicle formation⁶⁹. STING signalling in COPA-depleted HeLa cells therefore may occur from smaller Golgi fragments, rather than an intact Golgi complex. In line with our data, spontaneous Golgi accumulation of STING in cell lines overexpressing COPA mutants and COPA syndrome patient cells has recently been shown in other studies published while our manuscript was under review^37,38,67. Since Golgi dispersal was not observed in the complementary studies^9,37,38,67, this is likely a distinct feature of the COPA-deletion model system. Importantly, ligand-stimulated STING activation is retained in our COPA^deficient cells, suggesting that the observed Golgi fragmentation does not impair STING signalling⁷⁰.

In contrast to SAVI, we have demonstrated that aberrant type I IFN signalling in THP-1 cells lacking COPA and COPA-STING-adapter protein SURF4 requires upstream activation of cGAS, which normally protects cells from infections by sensing cytoplasmic DNA. This is in line with a previous study, which proposed tonic cGAS activation by low levels of cytoplasmic mitochondrial or genomic DNA as activators of STING translocation during the steady-state⁶⁷. Our data indicate that retrograde trafficking by COPI retrieves STING from the Golgi to prevent signalling as a key mechanism of negative regulation during homeostatic conditions. Following activation, STING binding to SURF4 and COPA is reduced³⁸, which results in accumulation at the Golgi and allows for interaction with downstream signalling molecules. Since the loss of function mutations in COPA reduce the COPI binding efficiency, steady-state Golgi-to-ER retrieval of the SURF4-STING complex is impaired and lowers the threshold for STING accumulation and signalling^9,37,38,67. This proposed mechanism is supported by the relatively high incomplete penetrance of clinical symptoms (around 25 %⁴) in individuals carrying COPA mutations, indicating the requirement of additional triggers or environmental factors to disrupt the balance of homeostatic STING circulation and induce disease onset. Although not yet identified, contributing co-factors could be infections or additional predisposing mutations in genes regulating ER stress pathways or other molecules involved in inflammatory signalling via cGAS/STING.

Furthermore, we observed increased levels of 2’3’-cGAMP in COPA^deficient THP-1 cells indicative of cGAS activation, which could be a secondary consequence of altered cellular homeostasis in COPA-deficiency. Further validation of these findings in model systems expressing COPA mutants is required, to exclude the possibility of Cas9-mediated cGAS activation in the here used experimental system⁷¹. cGAS activation as the primary consequence of COPA-deficiency seems less likely, since overexpression of COPA mutants in mouse embryonic fibroblasts and HEK293T cells induced aberrant STING signalling independent of cGAS^37,38,67, which demonstrates that the main pathway defect is caused by STING accumulation at the Golgi. Importantly, an activating stimulus appears to be required and provided either by overexpression of STING or baseline cGAS signalling^43,67. However, species-specific differences in the case of murine cell lines cannot be excluded^37,38,67.

Nevertheless, secondary activation of cGAS could further aggravate inflammation, since overactivation of cGAS by self-DNA has now been implicated in several inflammatory autoimmune pathologies. For example, Aicardi-Goutières syndrome and familial chilblain lupus are caused by mutations in three-prime repair exonuclease 1 (TREX1), ribonuclease H2 (RNaseH2) or sterile alpha motif domain and HD domain-containing protein 1(SAMHD1) that result in accumulation of genomic self-DNA in the cytoplasm via different mechanisms and therefore trigger cGAS activation and autoinflammation (reviewed in⁷²).

Another possibility is that cGAS activation could be the result of leakage of mitochondrial DNA into the cytoplasm^15,73,74. Within cells, ER and mitochondria form a structural and functional interactive network⁷⁵ and both organelles exchange metabolites, signalling molecules and ions through so called mitochondrial-associated membranes^76,77. COPA-deficiency-induced alterations in ER homeostasis may therefore impair mitochondrial integrity and lead to release of mitochondrial DNA which could subsequently activate cGAS^78,79. Intriguingly, cGAS has also been shown to undergo phase separation, which is described as droplet-like compartment formation for subsequent signalling⁸⁰. It is believed that this phenomenon is highly dependent on the availability of ions, such as Zinc (Zn²⁺) which are mainly stored in mitochondria and the ER⁸¹. Therefore, it is conceivable that increased ER stress activated by COPI-deficiency may result in uncontrolled release of Zn²⁺ ions into the cytoplasm, promoting the phase separation of cGAS and subsequent signalling⁸⁰. However, the mechanism of cGAS activation in COPA syndrome remains speculative and requires further investigation.

In our study, we show that the cGAS/STING pathway is activated upon deletion of different COPI-subunit proteins COPA, COPG1 or COPD, whereas deficiency of COPE does not induce inflammatory signalling. Therefore, one could speculate that there may be other interferonopathies associated with defective retrograde transport caused by lost function of COPI subunits other than COPA, that have not yet been described. Interestingly, loss of function mutations in COPB2 (COPβ’) or COPD (COPδ, encoded by ARCN1 gene) are linked to diseases associated with skeletal developmental defects and microcephalus formation^82,83. Given the manifestation of these conditions, an underlying IFNαβ signature may be present but undocumented. However similar to COPA syndrome, numerous other factors could be involved to determine whether a particular COPI deficiency results in a more pronounced developmental or inflammatory pathology.

A recent study reported a primary immunodeficiency disease associated with a novel homozygous loss of function mutation in COPG1 (K652E) and identified impaired retrograde trafficking of KDEL receptor-bound proteins and subsequently increased ER stress in activated B and T cells as the underlying disease-causing mechanism. Treatment with the chemical chaperon tauroursodeoxycholic acid (TUDCA), an ER stress relieving agent, was able to reverse the B and T cell dysfunction in COPG1^K652E mice upon exposure to pet store mice, however, IL-6 serum levels remained elevated⁸⁴, which suggests additional activation of an ER stress-independent inflammatory pathway. In our in vitro model, CRISPR/Cas9-mediated deletion of COPG1 resulted in spontaneous STING signalling. However, since levels of type I IFN and ISGs were not measured in COPG1 (K652E) patients and the clinical presentation does not overlap with symptoms of COPA syndrome, no conclusion about contribution of a STING-driven pathology can be drawn.

Interestingly, we demonstrate that deficiency of COPA and COPG1 subunits results in an inability to activate cGAS following stimulation with synthetic DNA ligands. This suggests defective innate immune defence mechanisms upon lost function of COPA and COPG1, which could perhaps contribute to immunodeficiency of COPG1 (K652E) patients. Although profound immunodeficiency has not been reported in COPA syndrome patients, recurrent respiratory and opportunistic infections were reported in individual cases^1,9,85,86. Since immune deficiency due to loss of cGAS/STING signalling is not described in the literature, it is not clear what pathology, if any, we should expect to see associated with COPI-mediated disease.

Overall, this study shows that the type I IFN signature described in COPA syndrome patients is caused by a spontaneous activation of the cGAS/STING pathway. This finding is particularly exciting in the context of pharmacological intervention. Originally, COPA syndrome patients have been treated with various combinations of immunosuppressive drugs including DMARDs (disease-modifying anti-rheumatic drugs), NSAIDs (nonsteroidal anti-inflammatory drugs) and biologics, which were only able to partially control the disease⁴. Recently published case reports show treatment of COPA syndrome patients with JAK1/2 inhibitors ruxolitinib, baricitinib and upadacitinib^7,8,9. Although the IFNαβ signature and joint inflammation were reduced successfully, patient lung function was only partially improved^7,8,9. Therefore, our study provides hope that targeting the cGAS/STING pathway directly, for example with a STING inhibitor such as H-151, may be more specific and thus proves a greater beneficial approach to control type I IFN-mediated symptoms in COPA syndrome.

Methods

Cell culture

Human embryonic kidney (HEK) 293 (CellBank Australia, code 85120602, (a gift from Stephen Mieruszynski, The Walter and Eliza Hall Institute of Medical Research (WEHI)), HEK293T cells (ATCC Cat. No. CRL-3216), HeLa cells (Curie Institute, Paris, a gift from Paul Gleeson, Department of Biochemistry and Molecular Biology, University of Melbourne) and immortalized bone marrow-derived macrophages (iBMDM, a gift from Daniel Simpson, WEHI, generated as described in⁸⁷) were cultured in DMEM (Gibco, Life Technologies) supplemented with 10 % Fetal Bovine Serum (FBS, Sigma-Aldrich) and 100 U/ml Penicillin/100 µg/ml Streptomycin (Sigma-Aldrich) in a humidified incubator at 37 °C and 10 % CO₂. Human monocytic THP-1 cells (ATCC, Cat. No. TIB-202) were maintained in RPMI-1640 (made inhouse, RPMI 1640 powder (Life Technologies), 23.8 mM Sodium Bicarbonate (NaHCO₃) (Merck), 1 mM Sodium Pyruvate (C₃H₃NaO₃) (Sigma-Aldrich), 100 U/ml Penicillin/100 µg/ml Streptomycin) supplemented with 10 % FBS and incubated in humidified atmosphere at 37 °C and 5 % CO₂. The clonal cGAS KO (cGAS^−/−) THP-1 cell line was generated by Mankan and colleagues as previously published⁴⁴.

CRISPR/Cas9 gene editing

COPA-, COPG1-, COPG2-, COPD-, COPE-deficient and MAVS^−/−, PKR^−/−, UNC93B1^−/−, NLRP3^−/−, STING^−/−, SURF4^−/− cells were generated using CRISPR/Cas9 gene editing as previously described⁸⁸. Cas9 was stably expressed using the FU-Cas9-mCherry plasmid (kind gift from M. Herold, Addgene plasmid #70182)⁸⁹ or lentiCRISPR v2 Cas9 (kind gift from F. Zhang, Addgene plasmid # 52961)^90,91 in THP-1 or HeLa cells, respectively. Single guide (sg) RNAs (sequences listed in Supplementary Table 1) were cloned into the Doxycycline (Dox)-inducible FgH1t-UTG or FgH1t-UTC construct (kind gift from M. Herold, Addgene plasmids #70183, #85551)⁸⁹. Gene deletion was induced by treatment with Dox (1 µg/ml, Sigma-Aldrich) for 72 hours (hrs), followed by 24 hrs resting period in some experiments. Protein or gene deletion was assessed by western blotting or quantitative Real-Time PCR (qRT-PCR). Stably Cas9-expressing THP-1 or HeLa cells were used as control cells and are referred to as parental cell line throughout this study.

Stable cell line generation

Stable STING-GFP-expressing HEK293T cells were generated via retroviral reconstitution following the method published previously⁹². Briefly, retrovirus-containing supernatant was generated by transient co-transfection of HEK293T cells (10 cm culture dish) with pMRX-hSTING-GFP (6 µg, kind gift from Nan Yan, Department of Immunology and Department of Microbiology, University of Texas), VSVg (4 µg) and gagpol (6 µg). Filtered (0.45 µm) supernatant was then used to infect HEK293T WT cells in presence of polybrene (8 µg/ml, Sigma-Aldrich), which were subsequently sorted for the low GFP-expressing population.

The reconstitution of cGAS^−/−/Cas9 and cGAS^−/−/COPA^deficient cell lines with pTRIP-CMV-GFP-FLAG-cGAS (kind gift from N. Manel, Addgene plasmid # 86675)⁴⁵ was performed via lentiviral transduction as previously described⁸⁸. Therefore, 1x10⁶ cells were incubated with 1 ml virus-containing supernatant and polybrene (8 µg/ml) and centrifuged for 3 hrs at 1055x g at 32 °C. Following 24 hrs incubation, virus-containing media was removed and STING inhibitor H-151 (2.5 µM, Life Chemicals) added in order to minimise cell death. After additional 24 hrs incubation, cells were subjected to FACS sorting for the GFP-low expressing population and grown to confluence.

QuikChange mutagenesis

The QuikChange Lightning Site-Directed Mutagenesis Kit (Cat. No. 210513, Agilent Technologies) was used to generate plasmids encoding the COPA syndrome patient mutations c.721 G > A (p.E241K) and c.698 G > A (p.R233H)¹ according to the manufacturer’s recommendations. As template, the pCMV6Entry-COPA-myc-DDK plasmid (Origene, Cat. No. RC214199, kind gift from A. Shum, Department of Medicine, University of California San Francisco) was used. Primer sequences are listed in Supplementary Table 2.

Cell transfection

For overexpression studies, HEK293 or HEK293T cells were initially seeded at 2.5x10⁵ or 2x10⁵ cells/well in a 6-well plate format, respectively and transiently transfected with 0.5-1 µg of total DNA as stated in the figure or figure legend. Transfection of all plasmids including pCMV6Entry-COPA-myc-DDK, pTRIP-CMV-GFP-FLAG-cGAS, pEF-BOS-mCitrine-STING and pEF-BOS-FLAG as an empty vector (EV) control (kindly provided by V. Hornung, LMU Munich), was performed with Lipofectamine 2000 (Life Technologies) reagent following the manufacturer’s instructions. After 24 hrs incubation, cells were lysed for immunoblot analysis.

Immunoprecipitation of mCitrine-STING for mass spectrometry-based quantitative proteomics

Immunoprecipitation (IP) experiments were performed similarly as previously described⁹³. Briefly, 3x10⁶ HEK293T cells were seeded in 10 cm culture dishes. The following morning cells were transiently transfected with 10 µg of either pEF-BOS EV control or pEF-BOS-mCitrine-hSTING plasmid DNA. After 48 hrs cells were lysed in 750 µl 1xNonidet P-40 [1% NP-40, 10% glycerol, 20 mM Tris-HCl pH 7.4, 150 mM NaCl, 1 mM ethylene glycol tetraacetic acid (EGTA), 10 mM sodium pyrophosphate (NaPPi), 5 mM sodium fluoride (NaF), 1 mM sodium orthovanadate (Na₃VO₄)] supplemented with 1 mM PMSF and 1 x cOmplete^TM Protease Inhibitor Cocktail (Cat. No. 11697498001, Roche Biochemicals, Mannheim, Germany). Whole cell lysates were clarified by centrifugation at 17,000x g for 10 minutes (min) at 4 °C. For each IP sample, 1 µg of mouse IgG2A monoclonal GFP antibody (Thermo Fisher Scientific, [E36] A-11120) was crosslinked to 50 µl of Protein A Dynabeads® (Thermo Fisher Scientific, 10002D) using 5 mM BS³ (Thermo Fisher Scientific) and incubated for 30 min at RT. The crosslinking reaction was quenched by adding 1 M Tris-HCl [pH 7.4]. Antibody-crosslinked Protein A Dynabeads® were thoroughly washed before 50 µl was then added to each IP sample and incubated on a rotator at 4 °C for 2 hrs. Beads were then washed four times with 1xNP-40 buffer using a DynaMag-2 magnetic holder (Thermo Fisher Scientific) before proteins were eluted with 0.5% SDS in PBS. Eluted protein material was subjected to tryptic digestion using the FASP method as previously described^94,95,96. Peptides were lyophilised using CentriVap (Labconco) prior to reconstituting in 60 μl 0.1% formic acid/2% acetonitrile. Peptide mixtures (2 μl) were separated by reverse-phase chromatography on a C18 fused silica column (I.D. 75 µm, O.D. 360 μm x 25 cm length) packed into an emitter tip (IonOpticks), using a nano-flow HPLC (M-class, Waters). The HPLC was coupled to an Impact II UHR-QqTOF mass spectrometer (Bruker) using a CaptiveSpray source and nanoBooster at 0.20 Bar using acetonitrile. Peptides were loaded directly onto the column at a constant flow rate of 400 nl/min with 0.1 % formic acid in MilliQ water and eluted with a 90 min linear gradient from 2 to 34% buffer B (99.9% acetonitrile and 0.1% formic acid). Mass spectra were acquired in a data-dependent manner including an automatic switch between MS and MS/MS scans using a 1.5 s duty cycle and 4 Hz MS1 spectra rate, followed by MS/MS scans at 8–20 Hz dependent on precursor intensity for the remainder of the cycle. MS spectra were acquired between a mass range of 200–2000 m/z. Peptide fragmentation was performed using collision-induced dissociation. Raw files consisting of high-resolution MS/MS spectra were processed with MaxQuant (version 1.6.6.0) for feature detection and protein identification using the Andromeda search engine⁹⁷ as previously described⁹⁸. Extracted peak lists were searched against the reviewed Homo sapiens (UniProt, March 2019) database as well as a separate reverse decoy database to empirically assess the false discovery rate (FDR) using strict trypsin specificity, allowing up to 2 missed cleavages. LFQ quantification was selected, with a minimum ratio count of 2. PSM and protein identifications were filtered using a target-decoy approach at an FDR of 1%. Only unique and razor peptides were considered for quantification with intensity values present in at least 2 out of 3 replicates per group. Statistical analyses were performed using LFQAnalyst⁹⁹ (https://bioinformatics.erc.monash.edu/apps/LFQ-Analyst/) whereby the LFQ intensity values were used for protein quantification. Missing values were replaced by values drawn from a normal distribution of 1.8 standard deviations and a width of 0.3 for each sample (Perseus-type). Protein-wise linear models combined with empirical Bayes statistics were used for differential expression analysis using Bioconductor package limma whereby the adjusted P value cutoff was set at 0.05 and log2 fold change cutoff set at 1. The Benjamini-Hochberg (BH) method of FDR correction was used. The mass spectrometry proteomics data have been deposited to the ProteomeXchange Consortium via the PRIDE (https://www.ebi.ac.uk/pride/archive/projects/PXD023135)¹⁰⁰ partner repository with the dataset identifier PXD023135. Localization of identified STING-interacting proteins to ER or Golgi compartments in Supplementary Data 1 was determined using the Gene Ontology database (https://www.ebi.ac.uk/QuickGO/, particularly cellular component terms).

Cell stimulation and inhibitors

THP-1 cells were stimulated with activators of the cGAS/STING pathway, such as HT-DNA (DNA sodium salt from herring testes (Sigma-Aldrich), 2 µg/ml, transfected), poly (dA:dT) (1 µg/ml, transfected, InvivoGen), 2’3’-c-di-AM(PS)₂ (Rp,Rp) (20 µM, InvivoGen). Transfections were performed using Lipofectamine 2000 (Life Technologies) and OptiMEM (Invitrogen) according to the manufacturer’s instructions.

STING inhibitor studies were performed during Dox treatment. Therefore, THP-1 cells were seeded at 8x10⁴ cells/6-well plate in 2 ml complete RPMI ( + Dox 1 µg/ml). After 34 hrs incubation, STING inhibitor H-151 (2.5 µM, Life Chemicals) or DMSO (Vehicle (Veh) control) was added and incubated for 11 hrs before the inhibitor was washed off and incubation with Dox continued until the 72 hr time point was reached when cells were harvested for analysis.

To assess induction of spontaneous signalling following cPLA2α inhibition in iBMDMs, 2x10⁵ cells were seeded in 400 µl complete DMEM (24-well plate format) and incubated with AACOCF3 (10 or 20 µM, Sapphire Bioscience) or DMSO for 6 hrs. To test inhibitor functionality, iNOS expression levels were investigated after overnight priming with IFNγ (50 ng/ml, 485-MI R&D Systems), followed by 30 min incubation with AACOCF3 (10 or 20 µM, Sapphire Bioscience) or DMSO and subsequent stimulation with LPS (25 ng/ml, LPS-SM Ultrapure, # tlrl-smlps, InvivoGen) for 6 hrs.

Immunoblotting

0.5–1x10⁶ cells were lysed in RIPA buffer (20 mM Tris-HCl (pH 7.3), 150 mM NaCl, 5 mM EDTA, 1% Triton X-100, 0.5% sodium deoxycholate, 0.1% SDS, 10% glycerol) supplemented with cOmplete^TM Protease Inhibitor Cocktail (Cat. No. 11697498001, Roche Biochemicals), 1 mM PMSF and phosphatase inhibitors (5 mM NaF, 10 mM NaPPi, 1 mM Na₃VO₄). Using Pierce centrifuge columns (Thermo Fisher Scientific), protein lysates were purified of DNA and subsequently mixed with SDS-PAGE sample buffer. Size-based protein separation was achieved by use of 4–12% SDS PAGE gels (Novex) and NuPAGE^TM MES SDS running buffer (Thermo Fisher Scientific). Proteins were then transferred onto a PVDF membrane (Immobilon^®-P Transfer Membrane, Millipore) via wet transfer and blocked in 5% skim milk/Tris-buffered saline (TBST) for 1 hr at room temperature (RT). Membranes were probed with primary antibody diluted in 5% skim milk/TBST or 5% bovine serum albumin (BSA)/TBST overnight at 4 °C: anti-COPA (Santa Cruz Biotechnology, clone H-3, sc-398099, dilution 1:1000), anti-COPD (Santa Cruz Biotechnology, clone E-12, sc-515549, dilution 1:1000), anti-COPE (Santa Cruz Biotechnology, clone A-4, sc-133195, dilution 1:1000), anti-phospho-STAT1 Tyr701 (Cell Signaling Technology, clone 58D6, #9167, dilution 1:1000), anti-phospho-TBK1/NAK Ser172 (Cell Signaling Technology, clone D52C2, #5483, dilution 1:1000), anti-phospho-IRF3 Ser386 (Abcam, ab76493, EPR2346, dilution 1:500), anti-STING (Cell Signaling Technology, clone D2P2F, #13647, dilution 1:1000), anti-STAT1 (Cell Signaling Technology, clone D1K9Y, #14994, dilution 1:1000), anti-TBK1/NAK (Cell Signaling Technology, #3013, dilution 1:1000), anti-cGAS (D1D3G, Cell Signaling Technology #15102, dilution 1:1000), anti-GFP (Life Technologies, #A11122, dilution 1:1000), anti-Myc-Tag (Cell Signaling Technology, clone 9B11, #2276, dilution 1:1000), anti-COPG (A-10, sc-393977, Santa Cruz Biotechnology, dilution 1:1000), anti-iNOS/NOS type II (BD Transduction Laboratories, #610329, dilution 1:1000), anti-NLRP3 (AdipoGen Life Sciences, Cryo-2, AG-20B-0014-C100, dilution 1:1000), anti-PKR (Santa Cruz Biotechnology, clone B-10, sc-6282, dilution 1:1000), anti-Cardif (AdipoGen Life Sciences, Adri-1, AG-20B-0004-C100, dilution 1:500) or anti-Actin-HRP (Santa Cruz Biotechnology, clone C4, sc-47778, dilution 1:10000).

Secondary antibody was incubated for 1 hr at RT (1:10,000, sheep anti-mouse IgG-HRP (Cat. No. NA931) or donkey anti-rabbit IgG-HRP (Cat. No. NA934), GE Healthcare). For development, Immobilon Forte Western HRP Substrate (Cat. No. WBLUF0500, Millipore) and the ChemiDoc Imaging touch system (BioRad) were used.

RNA isolation and quantitative real-time PCR

RNA was isolated using the ISOLATE II RNA Mini Kit (Cat. No. 52073, Bioline) following the manufacturer’s guidelines. The Superscript III Reverse transcriptase (Cat. No. 18080-085, Invitrogen) and oligo (dT) nucleotides (Cat. No. C110B-C, Promega) were used to reverse transcribe 1 µg of total RNA. Quantitative Real-Time PCR (qRT-PCR) was performed using Maxima SYBR Green/ROX qPCR Master Mix (Cat. No. K0223, Thermo Fisher Scientific) and the ViiA 7 Real-time PCR system (Thermo Fisher Scientific). qRT-PCR Primer sequences used in this study are listed in Supplementary Table 3. Samples were run in duplicates, normalized to housekeeper gene ACTIN and analysed using the ΔΔCt method. Data are presented as fold change relative to vehicle control or parental cell line as indicated in the figure.

ELISA

To measure the production of CXCL10 and IFNβ, THP-1 cells were seeded at 1.5x10⁵ cells per well into a 96-well plate after 48 hrs of Dox treatment. 24 hrs later, culture supernatants were collected and cytokine concentrations measured using the Human CXCL10/IP-10 Quantikine ELISA Kit (Cat. No. DIP100, R&D Systems) and VeriKine-HS Human IFN Beta Serum ELISA Kit (Cat. No. 41415, PBL Bioscience) following the manufacturer’s instructions.

The release of IFN-λ was measured following stimulation of the cGAS/STING pathway. Cells were cultured for 72 hrs in presence of Dox before being reseeded at 0.5x10⁵ cells/well into a 96-well plate format and stimulated with cGAS/STING pathway activators as described above. After 24 hrs incubation, cellular supernatants were collected and IFN-λ concentration measured using the IL-29/IL-28B (IFN-lamda 1/3) DuoSet ELISA (Cat. No. DY1598B, R&D Systems) according to the manufacturer’s instructions.

To measure 2’3’-cGAMP concentration at baseline or following cGAS activation, 1x10⁶ or 0.5x10⁶ cells were lysed in 50 µl Thermo M-PER mammalian protein extraction reagent (Cat. No. 78503, Thermo Fisher Scientific), respectively. Lysis was performed for 10 min at 4 °C with subsequent centrifugation for 15 min at maximum speed and 4 °C. Clarified lysates were analysed using the 2’3’-cGAMP ELISA Kit (Cat. No. 501700, Cayman Chemical) following the manufacturer’s instructions.

Immunofluorescence microscopy

Glass coverslips (18 mm x 18 mm, thickness 1½, Zeiss) were sterilised in 80% ethanol and placed in 6-well plates. After 72 hrs of Dox treatment, HeLa cells were seeded at 3x10⁵ cells/well in 2 ml complete growth medium and left to attach for 4–6 hrs. Following treatment of indicated wells with HT-DNA (2 µg/ml, transfected) for 2 hrs, cells were washed in 1xPBS and fixed in 2 ml ice-cold methanol for 15 min at −20 °C when stained for endogenous STING. Staining for ER (KDEL) and Golgi (GM130) markers was performed after fixation with 4% paraformaldehyde (Electron Microscopy Sciences) for 15 min at RT. The cells were thoroughly washed 3x in 1xPBS and blocked (5% normal goat serum, 0.3% Triton X-100, 1xPBS) for 1 hr at RT. Primary antibodies were diluted in antibody dilution buffer (1 % BSA, 0.3 % Triton X-100, 1xPBS) and incubated overnight at 4 °C in a wet chamber using the following antibodies and dilutions: anti-COPA (1:100, Santa Cruz Biotechnology, clone H-3, sc-398099), anti-COPG (1:100, Cat. No. 12393-I-AP, ProteinTech), anti-COPD (1:100, Cat. No. GTX630562, clone GT1318, GeneTex), anti-GM130-AF647 (1:500, ab195303, EP892Y, Abcam), anti-STING (1:100, Cell Signaling Technology, clone D2P2F, #13647), anti-KDEL (1:200, clone 10C3, ab12223, Abcam, (Supplementary Fig. 4, 5)) and anti-KDEL-AF568 (1:500, ab203421, EPR12668, Abcam, (Fig. 2f, Fig. 5b)). After 3 washes with 1xPBS, secondary antibodies (goat-anti-rabbit-AF647, Cat. No. A-21245, goat- anti-mouse-AF488, Cat. No. A-11001 (Invitrogen)) were diluted (1:1000) in antibody diluent and incubated for 1 hr at RT in the dark. Considering the host species of antibodies used for co-staining experiments, sequential or simultaneous staining was performed. Coverslips were washed 3x in 1xPBS and mounted onto microscopy slides using Fluoromount-G with DAPI (Cat. No. 00-4959-52, Thermo Fisher Scientific). Z-stack images were acquired using the Leica SP8 Resonant Scanning Confocal (Leica Microsystems) using Leica Application Suite X (LAS X) version 3.5.7.23225 (Supplementary Fig. 4, 5), the Zeiss LSM 880 NLO fast Airyscan Confocal (Zeiss) using ZEN 2.3 SP1 software (Fig. 2f) or the DeltaVision OMX-SR system (GE Healthcare) using softWoRx 7.0.0 software and immersion oil with an index of refraction of 1.518 and an Olympus PlanApo oil immersion objective lens with 60x/1.42 NA (Fig. 5b, c). Microscopical images were analysed with Fiji software (version 2.1.0) and are presented as maximum intensity projections. Quantification analysis (Fig. 5c) was performed using Fiji software by creation of surface for KDEL and GM130 and subsequent calculation of spatial overlay resulting in the percentage of KDEL signal inside the Golgi.

Patient PBMCs and FACS analysis

Human blood samples were collected after informed consent (ethical review board of Istituto Giannina Gaslini-Genova-Italy N. BIOL 6/5/04). Healthy control (HC) samples were collected from adult donors at the blood donation centre of the Istituto Giannina Gaslini and anonymized for population characteristics.

PBMCs from a COPA syndrome patient, previously reported in⁶ (blood sample collected at age 10 years), and two HC donors were isolated and treated with STING inhibitor H-151 (5 µM, InvivoGen) at 37 °C for 4 hrs. Cells were fixed with pre-warmed Fixation Buffer (BioLegend) at 37 °C for 15 min and permeabilized with pre-chilled True-Phos™ Perm Buffer (BioLegend) at −20 °C for 1 hr. Cells were then stained with CD3-APC mAb (SK7, BD Biosciences), CD14-FITC mAb (M5E2, BD Biosciences) and phospho-TBK1/NAK (Ser172) XP Rabbit mAb-PE (D52C2, Cell Signaling Technology) or Rabbit (DA1E) mAb IgG XP Isotype Control-PE (Cell Signaling Technology) at RT for 30 min. Samples were analyzed using the BD FACSCanto^TM flow cytometer (BD Biosciences) and FlowJo 10.5 software.

The monocyte population was firstly identified based on cell size and granularity and subsequently confirmed by gating for the CD14-positive/CD3-negative subpopulation (Supplementary Fig. 6a). Data for phosphorylated TBK1 (pTBK1) is presented as histogram showing mean fluorescence intensity (MFI) for the CD14-expressing monocyte population. Quantification (Fig. 3b) shows fold change of MFI (representing pTBK1) after H-151 treatment and was calculated using this formula:

\({{{{{\boldsymbol{fold}}}}}}\,{{{{{\boldsymbol{change}}}}}}\left({{{{{\boldsymbol{pTBK}}}}}}{{{{{\bf{1}}}}}}\right)={{{{{{\boldsymbol{MFI}}}}}}}^{{{{{{\boldsymbol{H}}}}}}-{{{{{\bf{151}}}}}}}-{{{{{{\boldsymbol{MFI}}}}}}}^{{{{{{\boldsymbol{isotype}}}}}}{{{{{\boldsymbol{ctrl}}}}}}}/{{{{{{\boldsymbol{MFI}}}}}}}^{{{{{{\boldsymbol{untreated}}}}}}}-{{{{{{\boldsymbol{MFI}}}}}}}^{{{{{{\boldsymbol{isotype}}}}}}{{{{{\boldsymbol{ctrl}}}}}}}\)

Statistical analysis

Unless stated otherwise in the figure legends, data are presented as mean of independent biological replicates showing individual data points. Error bars represent standard error of the mean (SEM), unless otherwise stated. Using the GraphPad Prism 8 software, the statistical comparison was made either by unpaired Student’s t-test, ratio paired Student’s t-test or one-way ANOVA with subsequent multiple comparison testing as stated in the figure legends. P values are indicated by numbers or as * P < 0.05, ** P < 0.01, *** P < 0.001, **** P < 0.0001.

Reporting summary

Further information on research design is available in the Nature Research Reporting Summary linked to this article.

Data availability

Data supporting the findings reported in this study are presented within the results section and the supplementary files. All graphs show individual data points pooled from replicate experiments. Raw data are available upon request from the corresponding author. The mass spectrometry proteomics data have been deposited to the ProteomeXchange Consortium via the PRIDE partner repository (http://proteomecentral.proteomexchange.org/cgi/GetDataset) with the dataset identifier PXD023135. Localization of identified STING-interacting proteins to ER or Golgi compartments in Supplementary Data 1 was determined using the Gene Ontology database (https://www.ebi.ac.uk/QuickGO/, particularly cellular component terms). Other databases used include Uniprot (https://www.uniprot.org/) and LFQAnalyst (https://bioinformatics.erc.monash.edu/apps/LFQ-Analyst/). Source data are available with this paper for Figs. 1a, d, 2b, d, 3c-e, 4a, 5c, d, 6a, d and supplementary figures 1, 2a-c, 3, 7, 8a and 10.

References

Watkin, L. B. et al. COPA mutations impair ER-Golgi transport and cause hereditary autoimmune-mediated lung disease and arthritis. Nat. Genet 47, 654–660 (2015).
Article CAS PubMed PubMed Central Google Scholar
Beck, R., Rawet, M., Wieland, F. T. & Cassel, D. The COPI system: molecular mechanisms and function. FEBS Lett. 583, 2701–2709 (2009).
Article CAS PubMed Google Scholar
Guan, Y. et al. Effective sirolimus treatment of 2 COPA syndrome patients. J. Allergy Clin. Immunology: Pract. 9, 999–1001.e1001 (2021).
Article Google Scholar
Frémond, M.-L. & Nathan, N. COPA syndrome, 5 years after: Where are we? Jt. Bone Spine 88, 105070 (2021).
Article CAS Google Scholar
Todd, D. J., Lee, A. H. & Glimcher, L. H. The endoplasmic reticulum stress response in immunity and autoimmunity. Nat. Rev. Immunol. 8, 663–674 (2008).
Article CAS PubMed Google Scholar
Volpi, S. et al. Type I interferon pathway activation in COPA syndrome. Clin. Immunol. (Orlando, Fla) 187, 33–36 (2018).
Article CAS Google Scholar
Fremond, M. L. et al. Use of ruxolitinib in COPA syndrome manifesting as life-threatening alveolar haemorrhage. Thorax 75, 92–95 (2020).
Article PubMed Google Scholar
Krutzke, S., Rietschel, C. & Horneff, G. Baricitinib in therapy of COPA syndrome in a 15-year-old girl. Eur. J. Rheumatol. 7, 1–4 (2019).
Google Scholar
Kato, T. et al. Augmentation of STING-induced type I interferon production in COPA syndrome. Arthritis Rheumatol. 73, 2105–115 (2021).
Ishikawa, H., Ma, Z. & Barber, G. N. STING regulates intracellular DNA-mediated, type I interferon-dependent innate immunity. Nature 461, 788–792 (2009).
Article ADS CAS PubMed PubMed Central Google Scholar
Jin, L. et al. MPYS, a novel membrane tetraspanner, is associated with major histocompatibility complex class II and mediates transduction of apoptotic signals. Mol. Cell Biol. 28, 5014–5026 (2008).
Article CAS PubMed PubMed Central Google Scholar
Zhong, B. et al. The adaptor protein MITA links virus-sensing receptors to IRF3 transcription factor activation. Immunity 29, 538–550 (2008).
Article CAS PubMed Google Scholar
Sun, W. et al. ERIS, an endoplasmic reticulum IFN stimulator, activates innate immune signaling through dimerization. Proc. Natl Acad. Sci. USA 106, 8653–8658 (2009).
Article ADS CAS PubMed PubMed Central Google Scholar
Li, Y., Wilson, H. L. & Kiss-Toth, E. Regulating STING in health and disease. J. Inflamm. 14, 11 (2017).
Article CAS Google Scholar
Li, T. & Chen, Z. J. The cGAS-cGAMP-STING pathway connects DNA damage to inflammation, senescence, and cancer. J. Exp. Med 215, 1287–1299 (2018).
Article CAS PubMed PubMed Central Google Scholar
Sun, L., Wu, J., Du, F., Chen, X. & Chen, Z. J. Cyclic GMP-AMP synthase is a cytosolic DNA sensor that activates the type I interferon pathway. Science 339, 786–791 (2013).
Article ADS CAS PubMed Google Scholar
Dobbs, N. et al. STING Activation by Translocation from the ER Is Associated with Infection and Autoinflammatory Disease. Cell host microbe 18, 157–168 (2015).
Article MathSciNet CAS PubMed PubMed Central Google Scholar
Balka, K. R. et al. TBK1 and IKKε Act Redundantly to Mediate STING-Induced NF-κB Responses in Myeloid Cells. Cell Rep. 31, 107492 (2020).
Article CAS PubMed Google Scholar
Liu, S. et al. Phosphorylation of innate immune adaptor proteins MAVS, STING, and TRIF induces IRF3 activation. Science 347, aaa2630 (2015).
Article PubMed CAS Google Scholar
Tanaka, Y. & Chen, Z. J. STING specifies IRF3 phosphorylation by TBK1 in the cytosolic DNA signaling pathway. Sci. Signal 5, ra20 (2012).
Article PubMed PubMed Central Google Scholar
Darnell, J. E. Jr. Studies of IFN-induced transcriptional activation uncover the Jak-Stat pathway. J. Interferon Cytokine Res.: Off. J. Int. Soc. Interferon Cytokine Res. 18, 549–554 (1998).
Article CAS Google Scholar
Kotenko, S. V. et al. IFN-λs mediate antiviral protection through a distinct class II cytokine receptor complex. Nat. Immunol. 4, 69–77 (2003).
Article CAS PubMed Google Scholar
Sudo, H. et al. Knockdown of COPA, identified by loss-of-function screen, induces apoptosis and suppresses tumor growth in mesothelioma mouse model. Genomics 95, 210–216 (2010).
Article CAS PubMed Google Scholar
Buttmann, M., Berberich-Siebelt, F., Serfling, E. & Rieckmann, P. Interferon-beta is a potent inducer of interferon regulatory factor-1/2-dependent IP-10/CXCL10 expression in primary human endothelial cells. J. Vasc. Res 44, 51–60 (2007).
Article CAS PubMed Google Scholar
Buttmann, M., Merzyn, C. & Rieckmann, P. Interferon-beta induces transient systemic IP-10/CXCL10 chemokine release in patients with multiple sclerosis. J. Neuroimmunol. 156, 195–203 (2004).
Article CAS PubMed Google Scholar
Li, X. et al. The tyrosine kinase Src promotes phosphorylation of the kinase TBK1 to facilitate type I interferon production after viral infection. Sci. Signal. 10, eaae0435 (2017).
Lau, L., Gray, E. E., Brunette, R. L. & Stetson, D. B. DNA tumor virus oncogenes antagonize the cGAS-STING DNA-sensing pathway. Science 350, 568–571 (2015).
Article ADS CAS PubMed Google Scholar
Pelka, K. et al. The Chaperone UNC93B1 Regulates Toll-like Receptor Stability Independently of Endosomal TLR Transport. Immunity 48, 911–922.e917 (2018).
Article CAS PubMed PubMed Central Google Scholar
Wu, J. et al. Cyclic GMP-AMP is an endogenous second messenger in innate immune signaling by cytosolic DNA. Science 339, 826–830 (2013).
Article ADS CAS PubMed Google Scholar
Ablasser, A. et al. cGAS produces a 2’-5’-linked cyclic dinucleotide second messenger that activates STING. Nature 498, 380–384 (2013).
Article ADS CAS PubMed PubMed Central Google Scholar
Ogawa, E., Mukai, K., Saito, K., Arai, H. & Taguchi, T. The binding of TBK1 to STING requires exocytic membrane traffic from the ER. Biochemical Biophysical Res. Commun. 503, 138–145 (2018).
Article CAS Google Scholar
Sun, M.-S. et al. TMED2 Potentiates Cellular IFN Responses to DNA Viruses by Reinforcing MITA Dimerization and Facilitating Its Trafficking. Cell Rep. 25, 3086–3098.e3083 (2018).
Article CAS PubMed Google Scholar
Ran, Y. et al. YIPF5 Is Essential for Innate Immunity to DNA Virus and Facilitates COPII-Dependent STING Trafficking. J. Immunol. 203, 1560–1570 (2019).
Article CAS PubMed Google Scholar
Gui, X. et al. Autophagy induction via STING trafficking is a primordial function of the cGAS pathway. Nature 567, 262–266 (2019).
Article ADS CAS PubMed Google Scholar
Zhang, B.-C. et al. STEEP mediates STING ER exit and activation of signaling. Nat. Immunol. 21, 868–879 (2020).
Article CAS PubMed PubMed Central Google Scholar
Szul, T. & Sztul, E. COPII and COPI Traffic at the ER-Golgi Interface. Physiology 26, 348–364 (2011).
Article CAS PubMed Google Scholar
Deng, Z. et al. A defect in COPI-mediated transport of STING causes immune dysregulation in COPA syndrome. J. Exp. Med. 217, e20201045 (2020).
Mukai, K. et al. Homeostatic regulation of STING by retrograde membrane traffic to the ER. Nat. Commun. 12, 61 (2021).
Article ADS CAS PubMed PubMed Central Google Scholar
Li, C. et al. Transmembrane Protein 214 (TMEM214) mediates endoplasmic reticulum stress-induced caspase 4 enzyme activation and apoptosis. J. Biol. Chem. 288, 17908–17917 (2013).
Article CAS PubMed PubMed Central Google Scholar
Saitoh, T. et al. Atg9a controls dsDNA-driven dynamic translocation of STING and the innate immune response. Proc. Natl Acad. Sci. USA 106, 20842–20846 (2009).
Article ADS CAS PubMed PubMed Central Google Scholar
Razi, M., Chan, E. Y. W. & Tooze, S. A. Early endosomes and endosomal coatomer are required for autophagy. J. Cell Biol. 185, 305–321 (2009).
Article CAS PubMed PubMed Central Google Scholar
Reus J. B., Trivino-Soto G. S., Wu L. I., Kokott K., Lim E. S. SV40 Large T Antigen Is Not Responsible for the Loss of STING in 293T Cells but Can Inhibit cGAS-STING Interferon Induction. Viruses 12, 137 (2020).
Ergun, S. L., Fernandez, D., Weiss, T. M. & Li, L. STING Polymer Structure Reveals Mechanisms for Activation, Hyperactivation, and Inhibition. Cell 178, 290–301.e210 (2019).
Article CAS PubMed Google Scholar
Mankan, A. K. et al. Cytosolic RNA:DNA hybrids activate the cGAS-STING axis. Embo j. 33, 2937–2946 (2014).
Article CAS PubMed PubMed Central Google Scholar
Raab, M. et al. ESCRT III repairs nuclear envelope ruptures during cell migration to limit DNA damage and cell death. Science 352, 359–362 (2016).
Article ADS CAS PubMed Google Scholar
Zhou, J. et al. Type III Interferons in Viral Infection and Antiviral Immunity. Cell. Physiol. Biochem. 51, 173–185 (2018).
Article CAS PubMed Google Scholar
Ank, N., West, H. & Paludan, S. R. IFN-lambda: novel antiviral cytokines. J. Interferon Cytokine Res.: Off. J. Int. Soc. Interferon Cytokine Res. 26, 373–379 (2006).
Article CAS Google Scholar
Munro, S. & Pelham, H. R. A C-terminal signal prevents secretion of luminal ER proteins. Cell 48, 899–907 (1987).
Article CAS PubMed Google Scholar
Lee, A.-H., Iwakoshi, N. N. & Glimcher, L. H. XBP-1 Regulates a Subset of Endoplasmic Reticulum Resident Chaperone Genes in the Unfolded Protein Response. Mol. Cell. Biol. 23, 7448–7459 (2003).
Article CAS PubMed PubMed Central Google Scholar
Ron, D. Translational control in the endoplasmic reticulum stress response. J. Clin. Invest 110, 1383–1388 (2002).
Article CAS PubMed PubMed Central Google Scholar
Duden, R., Kajikawa, L., Wuestehube, L. & Schekman, R. ϵ-COP is a structural component of coatomer that functions to stabilize α-COP. EMBO J. 17, 985–995 (1998).
Article CAS PubMed PubMed Central Google Scholar
Eugster, A., Frigerio, G., Dale, M. & Duden, R. COP I domains required for coatomer integrity, and novel interactions with ARF and ARF-GAP. Embo j. 19, 3905–3917 (2000).
Article CAS PubMed PubMed Central Google Scholar
Popoff, V., Adolf, F., Brügger, B. & Wieland, F. COPI budding within the Golgi stack. Cold Spring Harb. Perspect. Biol. 3, a005231 (2011).
Article PubMed PubMed Central CAS Google Scholar
Wegmann, D., Hess, P., Baier, C., Wieland, F. T. & Reinhard, C. Novel Isotypic γ/ζ Subunits Reveal Three Coatomer Complexes in Mammals. Mol. Cell. Biol. 24, 1070–1080 (2004).
Article CAS PubMed PubMed Central Google Scholar
Blagitko, N., Schulz, U., Schinzel, A. A., Ropers, H. H. & Kalscheuer, V. M. gamma2-COP, a novel imprinted gene on chromosome 7q32, defines a new imprinting cluster in the human genome. Hum. Mol. Genet 8, 2387–2396 (1999).
Article CAS PubMed Google Scholar
Futatsumori, M., Kasai, K., Takatsu, H., Shin, H. W. & Nakayama, K. Identification and characterization of novel isoforms of COP I subunits. J. Biochem 128, 793–801 (2000).
Article CAS PubMed Google Scholar
Moelleken, J. et al. Differential localization of coatomer complex isoforms within the Golgi apparatus. Proc. Natl Acad. Sci. USA 104, 4425–4430 (2007).
Article ADS CAS PubMed Google Scholar
Jain Goyal M., et al. A paralog-specific role of COPI vesicles in the neuronal differentiation of mouse pluripotent cells. Life Sci Alliance 3, e202000714 (2020).
Adolf, F. et al. Proteomic Profiling of Mammalian COPII and COPI Vesicles. Cell Rep. 26, 250–265 (2019). e255.
Article CAS PubMed Google Scholar
San Pietro, E. et al. Group IV phospholipase A(2)alpha controls the formation of inter-cisternal continuities involved in intra-Golgi transport. PLoS Biol. 7, e1000194 (2009).
Article PubMed CAS Google Scholar
de Figueiredo, P., Drecktrah, D., Katzenellenbogen, J. A., Strang, M. & Brown, W. J. Evidence that phospholipase A2 activity is required for Golgi complex and trans Golgi network membrane tubulation. Proc. Natl Acad. Sci. 95, 8642–8647 (1998).
Article ADS PubMed PubMed Central Google Scholar
Chuang, D. Y., Simonyi, A., Kotzbauer, P. T., Gu, Z. & Sun, G. Y. Cytosolic phospholipase A2 plays a crucial role in ROS/NO signaling during microglial activation through the lipoxygenase pathway. J. Neuroinflammation 12, 199 (2015).
Article PubMed PubMed Central CAS Google Scholar
Ng, C. Y. et al. A New Generation of Arachidonic Acid Analogues as Potential Neurological Agent Targeting Cytosolic Phospholipase A2. Sci. Rep. 7, 13683 (2017).
Article ADS PubMed PubMed Central CAS Google Scholar
Gonugunta, V. K. et al. Trafficking-Mediated STING Degradation Requires Sorting to Acidified Endolysosomes and Can Be Targeted to Enhance Anti-tumor Response. Cell Rep. 21, 3234–3242 (2017).
Article CAS PubMed PubMed Central Google Scholar
Liu, D. et al. STING directly activates autophagy to tune the innate immune response. Cell Death Differ. 26, 1735–1749 (2019).
Article CAS PubMed Google Scholar
Liu, Y. et al. Activated STING in a Vascular and Pulmonary Syndrome. N. Engl. J. Med. 371, 507–518 (2014).
Article CAS PubMed PubMed Central Google Scholar
Lepelley, A. et al. Mutations in COPA lead to abnormal trafficking of STING to the Golgi and interferon signaling. J. Exp. Med 217, e20200600 (2020).
Melki, I. et al. Disease-associated mutations identify a novel region in human STING necessary for the control of type I interferon signaling. J. allergy Clin. Immunol. 140, 543–552.e545 (2017).
Article CAS PubMed Google Scholar
Lippincott-Schwartz, J., Yuan, L. C., Bonifacino, J. S. & Klausner, R. D. Rapid redistribution of Golgi proteins into the ER in cells treated with brefeldin A: evidence for membrane cycling from Golgi to ER. Cell 56, 801–813 (1989).
Article CAS PubMed PubMed Central Google Scholar
Uhlorn B. L., Gamez E. R., Li S., Campos S. K. Attenuation of cGAS/STING activity during mitosis. Life Sci Alliance 3, e201900636 (2020).
Pépin, G. et al. Cre-dependent DNA recombination activates a STING-dependent innate immune response. Nucleic Acids Res 44, 5356–5364 (2016).
Article PubMed PubMed Central CAS Google Scholar
Zierhut, C. & Funabiki, H. Regulation and Consequences of cGAS Activation by Self-DNA. Trends Cell Biol. 30, 594–605 (2020).
Article CAS PubMed PubMed Central Google Scholar
Rongvaux, A. et al. Apoptotic caspases prevent the induction of type I interferons by mitochondrial DNA. Cell 159, 1563–1577 (2014).
Article CAS PubMed PubMed Central Google Scholar
White, M. J. et al. Apoptotic caspases suppress mtDNA-induced STING-mediated type I IFN production. Cell 159, 1549–1562 (2014).
Article CAS PubMed PubMed Central Google Scholar
Kornmann, B. et al. An ER-mitochondria tethering complex revealed by a synthetic biology screen. Science 325, 477–481 (2009).
Article ADS CAS PubMed PubMed Central Google Scholar
Vance, J. E. Phospholipid synthesis in a membrane fraction associated with mitochondria. J. Biol. Chem. 265, 7248–7256 (1990).
Article CAS PubMed Google Scholar
Malhotra, J. D. & Kaufman, R. J. ER stress and its functional link to mitochondria: role in cell survival and death. Cold Spring Harb. Perspect. Biol. 3, a004424 (2011).
PubMed PubMed Central Google Scholar
Bravo, R. et al. Endoplasmic reticulum: ER stress regulates mitochondrial bioenergetics. Int J. Biochem Cell Biol. 44, 16–20 (2012).
Article CAS PubMed Google Scholar
Wang, X. et al. ER stress modulates cellular metabolism. Biochem J. 435, 285–296 (2011).
Article CAS PubMed Google Scholar
Du, M. & Chen, Z. J. DNA-induced liquid phase condensation of cGAS activates innate immune signaling. Science 361, 704–709 (2018).
Article ADS CAS PubMed Google Scholar
Lu, Q., Haragopal, H., Slepchenko, K. G., Stork, C. & Li, Y. V. Intracellular zinc distribution in mitochondria, ER and the Golgi apparatus. Int J. Physiol. Pathophysiol. Pharm. 8, 35–43 (2016).
CAS Google Scholar
DiStasio, A. et al. Copb2 is essential for embryogenesis and hypomorphic mutations cause human microcephaly. Hum. Mol. Genet 26, 4836–4848 (2017).
Article CAS PubMed PubMed Central Google Scholar
Izumi, K. et al. ARCN1 Mutations Cause a Recognizable Craniofacial Syndrome Due to COPI-Mediated Transport Defects. Am. J. Hum. Genet 99, 451–459 (2016).
Article CAS PubMed PubMed Central Google Scholar
Bainter, W. et al. Combined immunodeficiency due to a mutation in the γ1 subunit of the coat protein I complex. The Journal of Clinical Investigation 131, e140494 (2021).
Jensson, B. O. et al. COPA syndrome in an Icelandic family caused by a recurrent missense mutation in COPA. BMC Med. Genet. 18, 129 (2017).
Article PubMed PubMed Central CAS Google Scholar
Taveira-DaSilva, A. M. et al. Expanding the phenotype of COPA syndrome: a kindred with typical and atypical features. J. Med Genet 56, 778–782 (2019).
Article CAS PubMed Google Scholar
De Nardo D., Kalvakolanu D. V., Latz E. Immortalization of Murine Bone Marrow-Derived Macrophages. In: Macrophages: Methods and Protocols (ed Rousselet G). Springer New York (2018).
Baker, P. J. & Masters, S. L. Generation of Genetic Knockouts in Myeloid Cell Lines Using a Lentiviral CRISPR/Cas9 System. Methods Mol. Biol. 1714, 41–55 (2018).
Article CAS PubMed Google Scholar
Aubrey, B. J. et al. An inducible lentiviral guide RNA platform enables the identification of tumor-essential genes and tumor-promoting mutations in vivo. Cell Rep. 10, 1422–1432 (2015).
Article CAS PubMed Google Scholar
Shalem, O. et al. Genome-scale CRISPR-Cas9 knockout screening in human cells. Science 343, 84–87 (2014).
Article ADS CAS PubMed Google Scholar
Sanjana, N. E., Shalem, O. & Zhang, F. Improved vectors and genome-wide libraries for CRISPR screening. Nat. Methods 11, 783–784 (2014).
Article CAS PubMed PubMed Central Google Scholar
Pokatayev, V. & Yan, N. Methods of Assessing STING Activation and Trafficking. Methods Mol. Biol. 1656, 167–174 (2017).
Article CAS PubMed PubMed Central Google Scholar
De Nardo, D. et al. Interleukin-1 receptor-associated kinase 4 (IRAK4) plays a dual role in myddosome formation and Toll-like receptor signaling. J. Biol. Chem. 293, 15195–15207 (2018).
Article PubMed PubMed Central Google Scholar
Wisniewski, J. R., Zougman, A., Nagaraj, N. & Mann, M. Universal sample preparation method for proteome analysis. Nat. Methods 6, 359–362 (2009).
Article CAS PubMed Google Scholar
Kedzierski, L. et al. Suppressor of cytokine signaling (SOCS)5 ameliorates influenza infection via inhibition of EGFR signaling. Elife 6, e20444 (2017).
Delconte, R. B. et al. CIS is a potent checkpoint in NK cell-mediated tumor immunity. Nat. Immunol. 17, 816–824 (2016).
Article CAS PubMed Google Scholar
Cox, J. et al. Andromeda: a peptide search engine integrated into the MaxQuant environment. J. Proteome Res 10, 1794–1805 (2011).
Article ADS CAS PubMed Google Scholar
Rautela, J. et al. Therapeutic blockade of activin-A improves NK cell function and antitumor immunity. Sci Signal 12, eaat7527 (2019).
Shah, A. D., Goode, R. J. A., Huang, C., Powell, D. R. & Schittenhelm, R. B. LFQ-Analyst: An Easy-To-Use Interactive Web Platform To Analyze and Visualize Label-Free Proteomics Data Preprocessed with MaxQuant. J. Proteome Res 19, 204–211 (2020).
Article CAS PubMed Google Scholar
Perez-Riverol, Y. et al. The PRIDE database and related tools and resources in 2019: improving support for quantification data. Nucleic Acids Res 47, D442–d450 (2019).
Article CAS PubMed Google Scholar

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Acknowledgements

We thank Thomas Hayman (Melbourne University, WEHI) and Fiona Moghaddas (Melbourne University, WEHI) for kindly providing the single guide RNAs for MAVS and STING, respectively. We thank Cynthia Louis (Melbourne University, WEHI) for providing human IL8 primers.

This work was supported by: Fellowships from the Australian National Health and Medical Research Council (NHMRC GNT2008699) (S.L.M.), HHMI-Wellcome International Research Scholarship 208694/Z/17/Z (S.L.M.), the Sylvia and Charles Viertel Foundation VTL2016F027 (S.L.M.), the National Health and Medical Research Council Early Career Fellowship (S.D. GNT1143412), the WEHI Centenary Fellowship (C.-H.Y.) and Ormond College’s Thwaites Gutch Fellowship in Physiology (C.-H.Y.), Italian Ministry of Health, Ricerca Corrente (M.Ga.). M,Ge., G.H. and T.Z. received funding by the Deutsche Forschungsgemeinschaft (DFG, German Research Foundation) under Germany’s Excellence Strategy – EXC2151 – 390873048 and TRR237 (G.H., T.Z.). A.S. is supported by the University of Melbourne through the International Research Training Program Scholarship and the DFG - GRK 2168. S.L.M. receives funding from Glaxosmithkline and IFM therapeutics. S.V. received financial support from the Italian Ministry of Foreign Affairs/Italian Health Ministry (PGR grant IN17GR10).

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These authors have contributed equally: Sophia Davidson, Seth L. Masters.

Authors and Affiliations

Inflammation Division, The Walter and Eliza Hall Institute of Medical Research, Parkville, VIC, 3052, Australia
Annemarie Steiner, Katja Hrovat-Schaale, Chien-Hsiung Yu, Pawat Laohamonthonkul, Cassandra R. Harapas, Dominic De Nardo, Sophia Davidson & Seth L. Masters
Department of Medical Biology, University of Melbourne, Parkville, VIC, 3010, Australia
Annemarie Steiner, Katja Hrovat-Schaale, Chien-Hsiung Yu, Pawat Laohamonthonkul, Cassandra R. Harapas, Ronnie Ren Jie Low, Laura F. Dagley, Sophia Davidson & Seth L. Masters
Institute of Structural Biology, University Hospital Bonn, 53127, Bonn, Germany
Annemarie Steiner & Matthias Geyer
Centre for Autoinflammatory Diseases and Primary Immunodeficiencies, IRCCS Istituto Giannina Gaslini, 16147, Genoa, Italy
Ignazia Prigione, Marco Gattorno & Stefano Volpi
Personalised Oncology Division, The Walter and Eliza Hall Institute of Medical Research, Parkville, VIC, 3052, Australia
Ronnie Ren Jie Low
Department of Anatomy and Developmental Biology, Monash Biomedicine Discovery Institute, Monash University, Clayton, VIC, 3168, Australia
Dominic De Nardo
Advanced Technology and Biology, The Walter and Eliza Hall Institute of Medical Research, Parkville, VIC, 3052, Australia
Laura F. Dagley
Center for Dynamic Imaging, The Walter and Eliza Hall Institute of Medical Research, Parkville, VIC, 3052, Australia
Michael J. Mlodzianoski & Kelly L. Rogers
Institute of Clinical Chemistry and Clinical Pharmacology, University Hospital Bonn, 53127, Bonn, Germany
Thomas Zillinger & Gunther Hartmann
Institute of Immunology, Philipps-University Marburg, BMFZ, 35043, Marburg, Germany
Thomas Zillinger
German Centre for Infection Research (DZIF), partner site Bonn-Cologne, 53127, Bonn, Germany
Gunther Hartmann
Centre for Innate Immunity and Infectious Diseases, Hudson Institute of Medical Research, Clayton, VIC, 3168, Australia
Michael P. Gantier
Department of Molecular and Translational Science, Monash University, Clayton, VIC, 3168, Australia
Michael P. Gantier
University of Genoa, 16126, Genoa, Italy
Stefano Volpi

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Annemarie Steiner
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Contributions

A.S., K.H.S., S.D., I.P., C.H.Y., D.D.N., L.F.D., C.R.H., P.L., M.J.M. and S.V. performed or assisted with experimentation. A.S., S.D., I.P., K.H.S, C.H.Y., D.D.N., L.F.D., C.R.H., P.L., R.R.J.L., M.J.M., K.R.R., T.Z., G.H. M.P.G., S.V., M.Ga, M.Ge, and S.L.M. were involved in experimental analysis and interpretation. All authors contributed to the writing of this manuscript.

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Correspondence to Seth L. Masters.

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M.Ga. declares consultancy and speakers fee from Novartis and SOBI. S.L.M. receives funding from IFM therapeutics and M.Ge. consults to IFM Therapeutics. The other authors declare no competing interests.

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Steiner, A., Hrovat-Schaale, K., Prigione, I. et al. Deficiency in coatomer complex I causes aberrant activation of STING signalling. Nat Commun 13, 2321 (2022). https://doi.org/10.1038/s41467-022-29946-6

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Received: 17 July 2020
Accepted: 05 April 2022
Published: 28 April 2022
DOI: https://doi.org/10.1038/s41467-022-29946-6

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