Glycans from microbial pathogens are well known pathogen-associated molecular patterns that are recognized by the host immunity; however, little is known about whether and how mammalian self-glycans activate the host immune response, especially in the context of autoimmune disease. Using biochemical fractionation and two-dimensional HPLC, we identify an abundant and bioactive free glycan, the Manβ1-4GlcNAc disaccharide in TREX1-associated autoimmune diseases. We report that both monosaccharide residues and the β1-4 linkage are critical for bioactivity of this disaccharide. We also show that Manβ1-4GlcNAc is produced by oligosaccharyltransferase hydrolysis of lipid-linked oligosaccharides in the ER lumen, followed by ENGase and mannosidase processing in the cytosol and lysosomes. Furthermore, synthetic Manβ1-4GlcNAc disaccharide stimulates a broad immune response in vitro, which is in part dependent on the STING-TBK1 pathway, and enhances antibody response in vivo. Together, our data identify Manβ1-4GlcNAc as a novel innate immune modulator associated with chronic autoimmune diseases.
The seminal work of immunologist Karl Landsteiner around 1900 identifying ABO blood groups led to the discovery that glycans can be powerful immunogens in humans. Later work demonstrated that innate immunity often recognizes glycans on pathogens to prevent infection. The mammalian innate immune system has evolved pattern recognition receptors (PRRs) to recognize microbial components termed pathogen-associated pattern molecules (PAMPs), which range from nucleic acids to lipids, peptides, and glycans1,2. This immune surveillance network can also be erroneously activated by self-ligands that mimic microbial PAMPs, thus leading to chronic autoimmune diseases. One such example is α-mannosidase-II deficiency, which causes production of hybrid N-glycans that bear immune-stimulatory mannose-dependent ligands that promote autoimmune disease in mice similar to lupus3.
We recently characterized TREX1, a gene associated with several recessive and dominant autoimmune and autoinflammatory diseases4. TREX1 is an ER-anchored DNase with two independent functions, cytosolic DNA clearance function through the N-terminal DNase domain and free glycan anabolism regulation function through the C-terminal ER domain5,6. Trex1−/− mice (loss of both DNase and glycan functions) develop severe early-onset systemic autoinflammatory disease with a short lifespan of 2–3 months5,7. In contrast, inactivating either DNase or glycan function alone in mice leads to less severe disease. For example, TREX1-D18N mutant mice disrupting only the DNase activity develop similar but significantly less severe disease phenotypes compared to Trex1−/− mice, and these mutant mice also survive much longer8. We previously showed that TREX1-V235fs mutant mice express a DNase-active TREX1 truncation that lack glycan regulatory function and develop serologic autoimmunity by producing free glycans and autoantibodies against non-nuclear self-protein antigens5,6.
The glycan regulatory function of TREX1 is associated with its C-terminus. Frame-shift mutations that truncate TREX1 C-terminus are associated with dominant late-onset immune disorders, such as systemic lupus erythematosus (SLE) and retinal vasculopathy with cerebral leukodystrophy (RVCL)9,10. We previously demonstrated that loss of TREX1 C-terminus dysregulates the mammalian oligosaccharyltransferase (OST) activity leading to accumulation of free oligosaccharides (fOS) in the cell, and that fOSs activate interferon-stimulated genes (ISGs) in macrophages5. However, the identities of the bioactive fOSs and how they are sensed by the immune system remain elusive. Here, we describe a major bioactive mammalian fOS, Manβ1-4GlcNAc, from Trex1-associated autoimmune disease. We also define structural requirements for bioactivity and immune profile of this self-derived disaccharide as well as its biogenesis and immune sensing pathway.
Identification of a bioactive mammalian disaccharide
We previously showed that fOS pools isolated from Trex1−/− cells are immunogenic when incubated with macrophages5. To determine the specific glycan structure(s) that are responsible for immune activation, we performed size exclusion fractionation of the Trex1−/− fOS pool and examined the bioactivity of each fraction on macrophages. We also analyzed each fraction by fluorophore-assisted carbohydrate electrophoresis (FACE). The majority of the fOS eluted in fractions #8-11 with larger structures eluting in fraction 8, medium structures in fraction 9, and smaller structures in fractions 10 and 11 (Fig. 1a). We then incubated fOS from each fraction as well as the non-fractioned fOS pool with RAW264.7 cells (a mouse macrophage cell line) for 24 h and measured immune activation. We chose Cxcl10 mRNA expression as our initial ‘immune activity’ readout because it was the most induced ISG in TREX1-V235fs RVCL patient lymphoblast cells5. Fraction 10 stimulated Cxcl10 the strongest; fraction 8 and 11 also appeared to be immunogenic but less potent compared to fraction 10 (Fig. 1a). The pattern of fOS fractionation and immune activity were highly consistent over four experiments. We also compared the immune profile of each fraction that contains fOS (#8-#11) by stimulating mouse bone marrow derived macrophages (BMDMs) and qRT-PCR array analysis of a panel of immune genes including type I interferon genes (IFN), IFN-stimulated genes (ISGs), inflammatory cytokine, and chemokine genes (Supplementary Fig. 1). We found that each fOS fraction stimulated a distinct immune profile. For example, fraction 10 stimulated the strongest Cxcl10 expression, whereas fraction 9 stimulated the strongest Il10 expression. Both fraction 10 and 11 stimulated Ifna and Cxcl2 expression to similar levels. These data suggest that multiple bioactive fOS structures exist in the Trex1−/− fOS pool.
To gain detailed structural information on these fOSs, we also analyzed WT and Trex1−/−fOS pool by two-dimensional HPLC analysis (i.e., size-fractionation HPLC followed by dual-gradient reversed-phase HPLC11). The most enriched fOS structures in Trex1−/− MEFs are paucimannose structures with one reducing-terminal GlcNAc (Man1-3GlcNAc) at ~20 fold higher levels than WT (Fig. 1b, Supplementary Fig. 2). Interestingly, the top three enriched glycan species match well with the predicted size of fOSs observed in fraction 10. We thus compared fraction 10 with chemically synthesized disaccharide (Manβ1-4GlcNAc, in-house, see Supplementary Methods), trisaccharide (Man2GlcNAc, in-house, see Supplementary Methods), and larger high-mannose glycans (Man5GlcNAc2 and Man9GlcNAc2, purchased from Sigma) by FACE. We found that the two major fOS species in fraction 10 co-migrate with the disaccharide (ManGlcNAc) and trisaccharide (Man2GlcNAc) standards (Fig. 1c). No other fractions contain detectable amount of disaccharide (ManGlcNAc) structure by FACE (Fig. 1c). Thus, we chose fraction 10 and the two fOS structures it contains for further analysis based on their high abundance and unique immune profile.
To see if any of these two fOS structures are bioactive, we stimulated RAW264.7 cells with increasing concentrations of the synthetic Man2GlcNAc and ManGlcNAc and measured Cxcl10 mRNA expression. Only ManGlcNAc induced Cxcl10 expression in a dose-dependent manner, while Man2GlcNAc lacked bioactivity in this assay (Fig. 1d). Together, these experiments suggest that the ManGlcNAc disaccharide is a bioactive glycan that is highly enriched in the Trex1−/− fOS pool.
Bioactivity is specific to only the Manβ1-4GlcNAc disaccharide
In our HPLC experiments we also analyzed Trex1−/− fOS pool after digestion with α-mannosidases, and we found that the ManGlcNAc disaccharide peak was not affected by digestion, suggesting that the glycosidic bond is a β linkage (Fig. 1b). To determine if the β linkage is critical for the bioactivity of the ManGlcNAc disaccharide, we treated cellular Trex1−/− fOS pool and the synthetic ManGlcNAc disaccharide with α- or β-mannosidase that selectively cleaves α- or β-mannosylated linkages, respectively, and assayed the digested glycan structures by FACE and bioactivity by stimulating macrophages and measuring Cxcl10 expression. α-Mannosidase treatment removed most of the high molecular weight fOSs from the Trex1−/− fOS pool but had no effect on the disaccharide band in the cellular fOS pool or synthetic ManGlcNAc disaccharide (Fig. 1e). In contrast, β-mannosidase digested the synthetic ManGlcNAc disaccharide as well as the disaccharide band in the fOS pool (Fig. 1e). β-mannosidase treatment reduced bioactivity of the fOS pool and bioactivity of the synthetic ManGlcNAc disaccharide, whereas α-mannosidase treatment had no effect (Fig. 1f). The residual activity in β-mannosidase-treated fOS pool indicates that other immunogenic fOS species also present in the fOS pool, consistent with our earlier observation that bioactivies were detected in multiple fractions from the fOS pool.
Glycosidic bonds can exist in two anomeric configurations, α or β. We next synthesized Manα1-4GlcNAc and compared its bioactivity to Manβ1-4GlcNAc (see Supplementary Methods). FACE analysis (which separates glycan based upon both oligosaccharide length and tertiary structural features that distinguish anomers and epimers) showed co-migration of Manβ1-4GlcNAc but not Manα1-4GlcNAc with the disaccharide band in the Trex1−/− fOS pool (Fig. 1g). Remarkably, only Manβ1-4GlcNAc, but not Manα1-4GlcNAc, stimulated Cxcl10 and Ifit1 expression in RAW267.4 cells, suggesting that the bioactivity was associated with the β1-4 linkage (Fig. 1h). We next compared Manβ1-4GlcNAc to other disaccharides that also contain the β1-4 linkage, such as Glcβ1-4GlcNAc and Galβ1-4GlcNAc (see Supplementary Methods). Again, only Manβ1-4GlcNAc disaccharide was immunogenic (Fig. 1i). We also examined the bioactivity of monosaccharides such as Man, GlcNAc, α-methyl mannose (Manα1-CH3), and β-methyl mannose (Manβ1-CH3). None of the monosaccharides were able to stimulate Cxcl10 expression to the extent of the Manβ1-4GlcNAc disaccharide in macrophages (Fig. 1j). Manβ1-CH3 had some activity but required 100 times higher concentration than Manβ1-4GlcNAc. We also analyzed fOS and immune profile of TREX1-V235fs mutant mouse BMDMs, and we found increased expression of Cxcl10 and several other immune genes as well as significantly elevated levels of Manβ1-4GlcNAc disaccharide (Supplementary Fig. 3A, 3B). Together, these results identify Manβ1-4GlcNAc as an abundant and bioactive mammalian self-glycan in TREX1-associated autoimmune disease cells. Both the Man and the GlcNAc, as well as the β1-4 linkage, are important for full bioactivity of this disaccharide at micromolar concentrations.
Biogenesis and cellular distribution of Manβ1-4GlcNAc
Oligomannose fOS can be generated from deglycosylation of ER-associated degradation (ERAD) substrates by N-glycanase NGLY1 or from the hydrolysis of lipid-linked oligosaccharide (LLOs) by the oligosaccharyltransferase (OST)12,13. We previously showed that absence of TREX1 or its C-terminus (e.g., TREX1-V235fs mutant) dysregulates the OST activity leading to accumulation of intracellular fOS5. To determine the source that leads to production of the Manβ1-4GlcNAc disaccharide, we used specific inhibitors that block either ERAD or OST activity and measured their effect on fOS production in Trex1−/− MEFs by FACE (Fig. 2a diagram). Inhibiting OST activity with aclacinomycin A (ACM5,14) led to significant reduction of Manβ1-4GlcNAc disaccharide as well as other high-mannose fOSs (Fig. 2b). In contrast, inhibiting of NGLY1 with Z-VAD-fmk15 had no effect on the Manβ1-4GlcNAc disaccharide or any other fOSs (Fig. 2c). We next examined ER translocation and glycan processing machinery in the lumen. Inhibiting ER glucosidases with castanospermine (CSN) blocks both the translocation of fOS to the cytoplasm as well as the progress through ERAD16,17, while inhibition of ER lumenal mannosidases with kifunensine (KIF) only affects misfolded protein tagging for ERAD18,19. Trex1−/− MEFs treated with CSN significantly reduced Manβ1-4GlcNAc disaccharide while treatment with KIF had no impact, suggesting that fOS derived from LLO hydrolysis are exported to the cytosol as large structures before trimming by ER luminal mannosidases (Fig. 2d, e and Supplementary Fig. 4A, 4B). We also tested cycloheximide (CHX, inhibits protein synthesis), MG132 (inhibits proteasomal degradation), and eeyarestatin I (ES1, inhibits ERAD), and none had any effect on the Manβ1-4GlcNAc disaccharide level in Trex1−/− MEFs (Supplementary Fig. 4C-4K). These data suggest that OST-hydrolyzed LLOs are precursors of the Manβ1-4GlcNAc disaccharide.
We next investigated how fOSs generated from LLOs get further processed into the Manβ1-4GlcNAc disaccharide. fOS derived from N-glycosylated proteins are processed by endo-β-N-acetylglucosaminidase (ENGase) in the cytosol. We thus examined the role of the ENGase pathway, which includes first trimming fOSs to Man5GlcNAc, transfer into the lysosomes and then further processed by α- and β-mannosidases into Manβ1-4GlcNAc disaccharide and monosaccharides20,21,22 (Fig. 3a diagram). ENGase knockdown by siRNA in Trex1−/− MEFs led to reduced Manβ1-4GlcNAc disaccharide levels as well as a corresponding increase in high molecular weight fOSs that co-migrated with previously characterized species in Engase−/− MEFs23 (Fig. 3b and Supplementary Fig. 5A). Conversely, MANBA (encodes β-mannosidase) knockdown led to increased Manβ1-4GlcNAc disaccharide level, further confirming the β linkage in the disaccharide and suggesting that β-mannosidase is the critical last enzyme in the pathway that breaks down the disaccharide (Fig. 3c and Supplementary Fig. 5B). Chloroquine treatment (CQ, lysosome neutralizer, thus inactivates β-mannosidase in the lysosome) also increased the disaccharide (Supplementary Fig. 5C, 5D). Because mammalian cells have multiple genes encoding α-mannosidase, we next treated Trex1−/− MEFs with a broad α-mannosidase inhibitor swainsonine (Swain24). Swainsonine completely eliminated the Manβ1-4GlcNAc disaccharide from Trex1−/− fOS and accumulated the Man3-5GlcNAc intermediates (Fig. 3d). We previously showed that ACM treatment inhibits OST activity and reduces ISG expression in Trex1−/− cells5. We next treated WT and Trex1−/− MEFs with increasing dose of swainsonine, and we observed dose-dependent decrease of ISG expression (Fig. 3e, 3f). These data suggest that LLO-derived fOSs move from the ER lumen to the cytosol followed by processing by ENGase and α-mannosidases to produce the Manβ1-4GlcNAc disaccharide. Also, interruption of Manβ1-4GlcNAc biogenesis in Trex1−/− cells reduces immune activation.
We next wanted to examine the cellular distribution of the mammalian Manβ1-4GlcNAc disaccharide. Treating the Trex1−/− MEFs with digitonin (10 μg/mL) that only permeabilized the plasma membrane25 led to lost of nearly half of the disaccharide, suggesting that a substantial fraction of Manβ1-4GlcNAc resides in the cytosol (Supplementary Fig. 5E). We also compared fOSs isolated from media and from cell lysates originated from the same tissue culture dish with a monolayer of healthy cells, and we found similar amount of the Manβ1-4GlcNAc disaccharide in both intracellular and extracellular compartments (Supplementary Fig. 5F). Together, these findings demonstrate that the bioactive Manβ1-4GlcNAc disaccharide resides in both intracellular and extracellular space.
Manβ1-4GlcNAc activates immune signaling via TBK1 and NF-κB
We performed RNA-seq to investigate the immune response activated by the synthetic Manβ1-4GlcNAc disaccharide or cellular Trex1−/− fOS pool in RAW267.4 macrophages. We found that 2044 genes were differentially expressed after the Manβ1-4GlcNAc disaccharide stimulation, 1131 genes after fOS pool stimulation, and 760 genes are shared between the two (Supplementary Fig. 6A). Ingenuity pathways analysis on the 760 shared genes revealed top pathways involved in T helper cell differentiation, antigen presentation, and upregulation of various chemokine genes from the CXCL family (Supplementary Fig. 6B). We validated several groups of immune genes including IFN, ISGs, inflammatory genes, and chemokine genes by qRT-PCR. The Manβ1-4GlcNAc disaccharide and fOS pool stimulated broad expression of immune genes including IFN and ISGs (as we observed before5) and many CXCL and CCL family chemokine genes (Fig. 4a).
To investigate whether Manβ1-4GlcNAc is detected by intracellular or extracellular receptors, we prepared permeabilized and non-permeabilized RAW267.4 cells and BMDMs and incubated them with Manβ1-4GlcNAc disaccharide. Primary macrophages such as BMDMs are more efficient at phagocytosis than macrophage cell lines such as RAW267.4 cells26. We found that Manβ1-4GlcNAc disaccharide only stimulated immune gene expression (e.g., Cxcl10, Ifit1) in permeabilized RAW267.4 cells and not in non-permeabilized RAW267.4 cells (Fig. 4b). In contrast, both permeabilized and non-permeabilized BMDMs showed dose-dependent and significant increase of immune gene expression after incubation with Manβ1-4GlcNAc disaccharide in the media, with permeabilizated BMDMs showing more robust response (Fig. 4c). Manβ1-4GlcNAc also induced increased cytokine and chemokine secretion in the media in permeabilized cells (Fig. 4d). Manβ1-4GlcNAc did not induce IL-10 expression in any of the conditions (Fig. 4b, c). These data suggest the possibility of an intracellular sensing pathway for Manβ1-4GlcNAc in macrophages.
We next sought to determine which immune pathway is required for sensing the Manβ1-4GlcNAc disaccharide. We chose a panel of knockout mice that are deficient in genes required for key innate immune signaling pathways (see Supplementary Fig. 6C for a diagram). TBK1 is a protein kinase required by several intracellular innate immune signaling pathways. IFN receptor 1 (IFNAR1) is required for type I IFN response. IRF3 and IRF7 are key transcription factors for IFN and ISG mRNA expression. MYD88 and TRIF are the two essential adaptor proteins required for TLR signaling. MAVS and STING are key non-redundant adaptor proteins for cytosolic RNA and DNA sensing pathways, respectively. We compared the response to the Manβ1-4GlcNAc disaccharide on BMDMs from wild-type, Tbk1Δ/Δ, Ifnar1−/−, Irf3−/−Irf7−/−, Myd88−/−Trif−/−, Mavs −/−, and Sting −/− mice. We found that wild-type, Ifnar1−/−, Myd88−/−Trif−/− and Mavs−/− BMDMs responded to the Manβ1-4GlcNAc disaccharide stimulation to similar levels. In contrast, Tbk1Δ/Δ BMDMs completely ablated immune response to Manβ1-4GlcNAc while Sting−/− and Irf3−/−Irf7−/− partially suppressed immune activation (Fig. 5a). To corroborate and extend on these findings, we pretreated wild-type BMDMs with TBK1 inhibitors (BX795 and Compound II), NF-κB inhibitors (TPCA-1 and dexamethasone), and JAK1/2 inhibitor ruxolitinib (inhibits type I IFN signaling), then stimulated with the Manβ1-4GlcNAc disaccharide. TBK1 and NF-κB inhibitors suppressed the activation of Cxcl10 and Cxcl2 while ruxolitinib had no effect (Fig. 5b). Taken together, these studies suggest that Manβ1-4GlcNAc-activated immune response is TBK1- and NF-κB-dependent but IFN- and TLR-independent.
Immune gene profile activated by Manβ1-4GlcNAc
Myeloid cells, which include macrophages, express an arsenal of carbohydrate binding proteins known as C-type lectins receptors (CLR) that function like PRRs and recognize a wide variety of glycan PAMPs. There are hundreds of lectins that can be potential candidate receptors for Manβ1-4GlcNAc disaccharide, making the individual knockdown approach impractical. It is also possible that Manβ1-4GlcNAc disaccharide represents a distinct type of bioactivity with its unique monovalent structure and micromolar activity concentration. Thus, we examined whether the Manβ1-4GlcNAc disaccharide stimulates an immune profile that can be matched to other non-mammalian bioactive glycans or non-glycan agonists. We stimulated BMDMs with Dectin-1 ligands (Chitosan, Chitin, Curdlan, and Zymosan), MGL ligand (Lewis-X)6, Dectin-2 ligands (β-Mannan, α-Mannan, Furfurman, and Lipoarabinomannan), and MCL/MINCLE ligand (Cord factor) as well as HT-DNA (herring testis DNA, activates cytosolic cGAS-STING-TBK innate immune pathway), LPS (activates TLR4 pathway), Manβ1-4GlcNAc disaccharide, and fOS pool. We then measured the expression of IFN, ISGs, inflammatory, and chemokine genes by qRT-PCR array. After hierarchical clustering that would group ligands with similar immune profiles, Manβ1-4GlcNAc disaccharide and the fOS pool emerged most similar to HT-DNA and chitosan (Figs. 6a, b). Both HT-DNA and chitosan activate the STING-TBK1 pathway in the cytosol27. We next analyzed the STING-TBK1 pathway in more detail by comparing a broader panel of immune genes activated by Manβ1-4GlcNAc disaccharide in WT, Tbk1Δ/Δ, and Sting−/− BMDMs. Tbk1Δ/Δ ablated all examined immune gene activation by Manβ1-4GlcNAc. Interestingly, Sting−/− eliminated expression of ISGs (e.g., Ifi44, Ifit1, Isg15, etc) but had little effect on chemokine genes (e.g., Ccl2, Ccl3, Cxcl2, etc. Note: Cxcl10 is both an ISG and a chemokine) in response to Manβ1-4GlcNAc (Fig. 6c).
Considering the similarities in immune profile between Manβ1-4GlcNAc and chitosan, we next compared two additional disaccharides, N,N′-diacetylchitobiose (GlcNAcβ1-4GlcNAc) and chitobiose (GlcNβ1-4GlcN), as well as their respective polymers, chitin and chitosan. Neither disaccharide structure stimulated Cxcl10 or Cxcl2 expression in BMDM at up to 1000 μM, while Manβ1-4GlcNAc stimulated significant increased immune response at 100 μM. Chitosan, but not chitin, also stimulated robust Cxcl10 expression in BMDMs at very low concentration (0.1 μM). These data further support the unique structure and immune activity of Manβ1-4GlcNAc in comparison to other disaccharides. It also raises the possibility that polymeric form of Manβ1-4GlcNAc (e.g., similar to chitobiose versus chitosan) could have more potent immune activities.
Manβ1-4GlcNAc enhances antibody response in vivo
To further substantiate our findings, we stimulated BMDCs with Manβ1-4GlcNAc and found increased secretion of multiple chemokines, including Cxcl10, Ccl2, Ccl3 (Fig. 7a). We did not detect activation markers of BMDCs such as MHC-II, CD86, CD80 after Manβ1-4GlcNAc stimulation (Supplementary Fig. 7A, B). We also stimulated wild-type splenocytes ex vivo with the disaccharide and did not observe direct activation of either T or B cells (Supplementary Fig. 7C). All glycans are chemically synthesized and confirmed by structural analysis (Supplementary Figs. 8–20). We next tested the activity of Manβ1-4GlcNAc in vivo. We first transferred mixed OT1 and OT2 splenocytes into wild-type mice, then immunized subcutaneously with either vehicle, OVA alone, OVA + MG (Manβ1-4GlcNAc) or OVA + LPS on day 0, 7, and 14. Seven days after the last immunization, we collected serum for antibody analysis and splenocytes for IFNγ ELISPOT assay. We detected significantly higher OVA-specific IgG1 in OVA + MG-treated mice compared to those treated with OVA alone, suggesting that Manβ1-4GlcNAc enhanced B cell-mediated antibody response in vivo (Fig. 7b). Manβ1-4GlcNAc did not significantly enhance T cell response (Fig. 7b). Interestingly, we previously showed that TREX1-V235fs mice develop serologic autoimmunity with increased autoantibody production in the serum and enhanced immune gene expression in cells6. Thus, together, our in vitro and in vivo data suggest that Manβ1-4GlcNAc activates a broad immune profile in DCs and macrophages that are mediated in part through STING and other immune sensing pathway(s) that converge on TBK1, which lead to enhanced antibody response in vivo.
Mammalian self-nucleic acids are well known for their causal association with autoimmune disease. Much less is known about whether and how mammalian self-glycans also activate immune responses associated with autoimmunity. Here, we identified a bioactive fOS, the Manβ1-4GlcNAc disaccharide, that is produced by OST hydrolysis of LLOs in the ER lumen, processed by ENGase and mannosidases in the cytosol, and sensed in part by the cytosolic STING-TBK1-dependent innate immune pathway.
We found that the bioactivity of Manβ1-4GlcNAc disaccharide requires both monosaccharides as well as the β1-4 linkage, and this disaccharide is surprisingly active in comparison to other disaccharide we tested. The immune profile of Manβ1-4GlcNAc is remarkably similar to that of chitosan, which also activates the STING-TBK1 pathway27. Structurally distinct chitosans also promote IFN or inflammasome responses28. Interestingly, chitosan is a polysaccharide of β1-4-linked glucosamine (GlcN), and we found that GlcNβ1-4GlcN disaccharide alone does not have detectable immune activities even at high concentrations. Thus, given the impressive bioactivity of Manβ1-4GlcNAc, we expect that a polysaccharide containing repeats of Manβ1-4GlcNAc could potentially have very potent immune-stimulating activities.
We further defined the immunogenicity of the Manβ1-4GlcNAc disaccharide in vivo and in vitro. Using an immunization experiment with the model antigen OVA, we found that the disaccharide stimulated significantly increased antibody response but not T cell response, although the overall response is relatively weak. This is not surprising because: (1) The disaccharide is only one of several immunogenic glycans we identified; (2) Disaccharides are not expected to be highly immunogenic, and polysaccharides are. (3) The receptor for Manβ1-4GlcNAc is likely intracellular. Nonetheless, the enhanced antibody response is consistent with our previous findings that TREX1-V235fs mice develop serologic autoimmunity6. We also defined the cell subsets affected by Manβ1-4GlcNAc. Myeloid cells such as macrophages are directly activated by Manβ1-4GlcNAc. DCs do respond to Manβ1-4GlcNAc although to a less extent comparing to macrophages. Manβ1-4GlcNAc does not directly activate T and B cells when stimulated ex vivo. Thus, it is likely that Manβ1-4GlcNAc primarily affects myeloid cells such as macrophages (through intracellular receptors) and induces expression of inflammatory cytokines and chemokines that promote a predominant B cell-mediated antibody response. Future studies depleting these myeloid populations will help define their function in vivo.
Although the Manβ1-4GlcNAc disaccharide has not been found on pathogens as a PAMP, it has been associated with microbial metabolic activity for colonization or infection29,30. Bacterial pathogens digest mammalian N-glycans on cells to facilitate infection. In doing so, many bacterial pathogens produce the Manβ1-4GlcNAc disaccharide and other fOSs, which are typically considered as by-products31. Therefore, it is possible that these mammalian fOSs produced during infection could function as danger-associated molecular patterns (DAMPs) that alert the host of the infection. In support of this notion, our previous work has demonstrated that fOSs are produced when cells are undergoing ER stress or infected with herpes simplex virus 1 (HSV-1)32.
Defects in cellular glycan processing enzymes can lead to chronic immune disorders. α-mannosidase-II deficiency leads to production of N-glycans that bear immune-stimulatory mannose-dependent ligands that promote autoimmune diseases similar to lupus3. Deficiency of β-mannosidase in humans and mice cause a chronic disease called β-mannosidosis, which causes accumulation of the Manβ1-4GlcNAc disaccharide in multiple disease-affected tissues33,34 and neuropathological characteristics that resemble inflammation35,36. We previously showed that Trex1-deficiency or fs mutations dysregulate the OST complex leading to production of immunogenic high-mannose fOS5,6. Our data here further show that multiple bioactive fOS species are produced when OST is dysregualted, potentially each with distinct immune profile. Thus, our data reveal an exciting possibility for distinct mammalian fOSs, such as Manβ1-4GlcNAc defined here, to play a role in autoimmune disease pathogenesis. Lastly, our inhibitor studies targeting the biogenesis or immune sensing pathways of Manβ1-4GlcNAc demonstrated several avenues of therapeutics for treating TREX1-fs RVCL, β-mannosidosis, and potentially other chronic autoimmune diseases.
Cells, antibodies, and reagents
MEFs, RAW264.7, BMDM, and BMDC were maintained in Dulbecco’s modified Eagle’s medium (DMEM) with 10% (v/v) heat-inactivated fetal bovine serum (FBS), with 2 mM L-glutamine, 10 mM HEPES, and 1 mM sodium pyruvate (complete DMEM) with the addition of 100 U/ml penicillin, 100 mg/ml streptomycin except MEFs and cultured at 37 °C with 5% CO2. MEFs, BMDM, and BMDCs were generated from WT C57BL/6 mice37. RAW264.7 cells were obtained from ATCC. Antibodies used in this study include anti-ubiquitin (rabbit, 1:1000 dilution, P4D1, Cell Signaling Technology), anti-Tubulin (mouse, 1:20,000 dilution, B-5-1-2, Sigma–Aldrich), anti-LC3 (rabbit, 1:1000 dilution,ab48394, Abcam), anti-STING (rabbit, 1:500 dilution, D2P2F, Cell Signaling), anti-GAPDH (rabbit, 1:1000 dilution, sc-25778, Santa Cruz), anti-Rab5 (rabbit, 1:1000 dilution,ab109534, Abcam), and anti-HMGB1 (rabbit; 1:2,000 dilution;ab18256; Abcam). The inhibitors used in this study are ACM (1 uM, Santa Cruz), Z-VAD-fmk (30 uM, BD), Q-VD-OPh (50 uM, BD), CSN (100 uM, Sigma–Aldrich), Kif (100 uM, Sigma–Aldrich), ES1 (10 uM, Sigma–Aldrich), CHX (10 ug/ml, Sigma–Aldrich), MG132 (1 uM, Sigma–Aldrich), Swain (10 uM, Tocris), Clq (10 uM, Sigma–Aldrich), Compound II (1 uM, UTSW), BX759 (1 uM, Invivogen), Ruxolitinib (1 uM, Invivogen), Dexamethasone (100 nM, Invivogen), and TPCA1 (1 uM, Sigma–Aldrich). The ligands used to stimulate macrophages are GalGlcNAc (Sigma–Aldrich), Mannose (Sigma–Aldrich), GlcNAc (Sigma–Aldrich), Manα1-CH3 (Sigma–Aldrich), Manβ1-CH3(Santa Cruz), LPS (100 ng/ml, Invivogen), htDNA (1 ug, Sigma–Aldrich), Chitosan (10 ug/ml, Invivogen), Chitin (10 ug/ml, Sigma–Aldrich), Curdlan (10 ug/ml, Invivogen), Zymosan (10 ug/ml, Invivogen), LeX (10 ug/ml,Sigma–Aldrich), β-Mannan (10 ug/ml, Megazyme), α-Mannan (10 ug/ml, Sigma–Aldrich), Furfurman (10 ug/ml, Invivogen), Lipoarabinomannan (1 ug/ml, Invivogen), and Cord factor (1 ug/ml, Invivogen). The alpha-mannosidase used in Fig. 1b is alpha(1-2,3,6) mannosidase from Jack bean (Prozyme, catalog number GKX-5010). It can remove all alpha-mannose from high-mannose-type glycans (unless they are capped by glucose). All uncropped western blot scans are in Source Data.
Fluorophore-assisted carbohydrate electrophoresis (FACE) analysis was done as follows (also described in ref. 5). Briefly, MEFs were plated at 75–80% confluency and transfected (RNAiMAX, Thermo Fisher) with the ENGase siRNA (Sigma–Aldrich) or treated with inhibitors for 24 h and disrupted with methanol the next day. The methanol disrupted cells or the lyophilized media were subject to a three-phase (aqueous, interface, and organic) extraction, which yields an aqueous fraction containing neutral fOS (desalted by ion exchange chromatography) and an interface fractions, which was extracted with chloroform:methanol:water (10:10:3) to isolate total proteins that was used to normalize the loading of labeled fOS to gels, immunoblotting and for the isolation of N-linked glycans by PNGase F digestion (New England Biolabs). Isolated glycans (fOS and digested N-glycans) were conjugated with 7-amino-1,3-naphthalenedisulfonic acid (ANDS, AnaSpec) and subjected to reductive amination with NaBH3CN (Sigma–Aldrich) for 24 h at 37 °C. Labeled fOS and digested N-glycans were resolved on an oligosaccharide profiling gel, with 10 pmol of glucose oligomers (ranging from four to seven glucosyl residues) and 100 pmol of Man9GlcNAc2 (Sigma–Aldrich), Man5GlcNAc2 (Sigma–Aldrich), Man2GlcNAc and ManGlcNAc as standards. Gels were visualized using a UVP Chemidoc-ItII scanner and quantified with VisionWorks software.
RNA isolation, RNA sequencing, and quantitative RT-PCR
Approximately 0.5 × 106 RAW264.7 cells or BMDM were seeded in a 12-well plate and stimulated the next day with the indicated ligands for 24 h by addition to the media or permeabilization as describe in ref. 5 and ref. 25, respectively. Total RNA was subsequently isolated with TRI reagent (Sigma–Aldrich) as indicated by the manufacturer and cDNA was synthesized with iScript cDNA synthesis kit (Bio-Rad) and analyzed using a Bio-Rad CFX qRT-PCR. PCR array of immune gene groups was performed using PrimePCR Array plates using iTaq Universal SYBR Green Supermix (Bio-Rad). RNA-Seq was performed as previously described in ref. 37. Pathway analysis was done using the Ingenuity Pathway Analysis software (Qiagen). Primers used in this study are in Supplementary Table 1.
Gel-filtration chromatography and mannosidase digestion
A 0.5 × 20 cm column was packaged with 6 ml of the BioGel P4 resin (Bio-Rad) and conditioned with a 25 mM NH4CH3COO (Sigma–Aldrich) buffer. Ten nanomoles of the total fOS were loaded into the column and 24 fractions (500 ul per fraction) were collected. Sample were dried in vacuum and later resuspended in water and desalted by ion exchange chromatography. Ten percent of each fraction was collected for FACE analysis, and the remaining 90% was divided in half and used for macrophage stimulation in biological duplicates. For the mannosidase digestion, 10 nmol of fOS or the synthetic ManGlcNAc disaccharide were treated with 40 U of α1-6 mannosidase (New England Biolabs) and 32 U of α1-2, 3 mannosidase (New England Biolabs). Samples were then mixed with 3 volumes of cold ethanol and centrifuged at 20,000 × g for 20 min at 4 °C. The supernatant was dried in vacuum and later resuspended in water and desalted by ion exchange chromatography. Ten percent of the digested product was collected for FACE analysis and the remaining 90% was divided in half and used for macrophage stimulation in biological duplicates.
Structural analysis of free oligosaccharides
Free oligosaccharides in wild-type and Trex1−/− cells were prepared as follows (also described in ref. 11). Briefly, 0.32 g of wild-type cells or 0.14 g of Trex1−/− cells were resuspended with 800 ul of homogenization buffer (10 mM Hepes/NaOH buffer (pH 7.4) containing 5 mM dithiothreitol, 250 mM mannitol, 1 mM EDTA, 1 x complete protease inhibitor cocktail (EDTA-free; Roche Applied Science), and 1 mM of Pefabloc (Roche Applied Science)). After the cells were homogenized in a Potter-Elvehjem homogenizer, the supernatant of 100,000 × g centrifuged samples was obtained. The supernatant fractions were mixed with 3 volumes of cold ethanol, followed by centrifugation at 17,000 × g for 20 min at 4 °C. The supernatants were dried, and desalted using a PD-10 column (GE Healthcare). The free oligosaccaharide fraction thus obtained were subjected to fluorescence-labeling with 2-aminopyridine (PA). Detailed methods for PA-labeling, as well as removal of excess reagents were described previously38. Separation of PA-labeled free oligosaccaharides were carried out first by size-fractionation using a Shodex NH2P-50 3E column (3.0 × 250 mm; Shodex, Tokyo, Japan) as described previously39. Each PA-labeled glycans were further separated by a dual-gradient HPLC as described previously40. Structures of each PA-glycan isolated were confirmed by a co-elution of standard PA-glycans as prepared previously11.
Mouse immunization study
C57BL/6 mice were transferred with mixed splenocytes (2 × 106 for each) from OT1 and OT2 transgenic mice on day 1, and then immunized subcutaneously with 100 µg OVA together with/without 100 μg Manβ1-4GlcNAc or 20 μg LPS on day 0, 7, and 14. Seven days after the last immunization, serum of treated mice was collected for antibody detection with ELISA, and splenocytes were isolated for IFNγ ELISPOT assay. Serum anti-OVA IgG1 was measured using an ELISA kit per manufacturer’s protocol (Cayman #500830). Spleens from treated mice were processed into single cell suspensions and resuspended in RPMI 1640 medium supplemented with 10% fetal bovine serum, 2 mmol/l L-glutamine, 100 U/ml penicillin, and 100 μg/ml streptomycin. 5 × 105 splenocytes were used for the IFNγ ELISPOT assay, 5 μg /ml of OVA (257-264), OVA (323-339), or SIY (SIYRYYGL) peptide were used to re-stimulate the antigen specific T cells. IFN-γ production was determined 48 h after of incubation with an IFN-γ ELISPOT assay kit according to the manufacturer’s protocol (BD Biosciences). The visualized spots were enumerated with the CTL-ImmunoSpot® S6 Analyzer (Cellular Technology Limited).
All mice were housed in pathogen-free barrier facility in UT Southwestern Medical Center. Both male and female 6–8 week old mice were used. All mice were on C57BL/6 background. Five mice per group were used in each repeat of the experiment. All mouse experiments were approved by ICUAC in UT Southwestern Medical Center.
See Supplementary Methods.
Further information on research design is available in the Nature Research Reporting Summary linked to this article.
All raw data, original gel images, processed RNA-seq data and pathway analysis are included in the Source Data file. Original RNA-seq data are deposited at NCBI gene expression omnibus (GEO, accession number GSE129677).
Sancho, D. & Reis e Sousa, C. Signaling by myeloid C-type lectin receptors in immunity and homeostasis. Annu. Rev. Immunol. 30, 491–529 (2012).
Rabinovich, G. A., van Kooyk, Y. & Cobb, B. A. Glycobiology of immune responses. Ann. N. Y. Acad. Sci. 1253, 1–15 (2012).
Green, R. S. et al. Mammalian N-glycan branching protects against innate immune self-recognition and inflammation in autoimmune disease pathogenesis. Immunity 27, 308–320 (2007).
Yan, N. Immune diseases associated with TREX1 and STING dysfunction. J. Interferon Cytokine Res. 37, 198–206 (2017).
Hasan, M. et al. Cytosolic nuclease TREX1 regulates oligosaccharyltransferase activity independent of nuclease activity to suppress immune Activation. Immunity 43, 463–474 (2015).
Sakai, T. et al. DNase-active TREX1 frame-shift mutants induce serologic autoimmunity in mice. J. Autoimmun. 81, 13–23 (2017).
Gall, A. et al. Autoimmunity initiates in nonhematopoietic cells and progresses via lymphocytes in an interferon-dependent autoimmune disease. Immunity 36, 120–131 (2012).
Grieves, J. L. et al. Exonuclease TREX1 degrades double-stranded DNA to prevent spontaneous lupus-like inflammatory disease. Proc. Natl Acad. Sci. USA 112, 5117–5122 (2015).
Lee-Kirsch, M. A. et al. Mutations in the gene encoding the 3’-5’ DNA exonuclease TREX1 are associated with systemic lupus erythematosus. Nat. Genet. 39, 1065–1067 (2007).
Richards, A. et al. C-terminal truncations in human 3′-5′ DNA exonuclease TREX1 cause autosomal dominant retinal vasculopathy with cerebral leukodystrophy. Nat. Genet. 39, 1068–1070 (2007).
Seino, J. et al. Basal autophagy is required for the efficient catabolism of sialyloligosaccharides. J. Biol. Chem. 288, 26898–26907 (2013).
Harada, Y. et al. Eukaryotic oligosaccharyltransferase generates free oligosaccharides during N-glycosylation. J. Biol. Chem. 288, 32673–32684 (2013).
Harada, Y., Hirayama, H. & Suzuki, T. Generation and degradation of free asparagine-linked glycans. Cell. Mol. life Sci. 72, 2509–2533 (2015).
Bennett, D. C. et al. High-throughput screening identifies aclacinomycin as a radiosensitizer of EGFR-mutant non-small cell lung cancer. Transl. Oncol. 6, 382–391 (2013).
Kessler, B., Spooner, E., Korbel, G. A., Ploegh, H. L. & Misaghi, S. z-VAD-fmk inhibits peptide:N-glycanase and may result in ER stress. Cell Death Differ. 13, 163 (2005).
Haga, Y., Totani, K., Ito, Y. & Suzuki, T. Establishment of a real-time analytical method for free oligosaccharide transport from the ER to the cytosol. Glycobiology 19, 987–994 (2009).
Hebert, D. N., Lamriben, L., Powers, E. T. & Kelly, J. W. The intrinsic and extrinsic effects of N-linked glycans on glycoproteostasis. Nat. Chem. Biol. 10, 902–910 (2014).
Moore, S. Transport of free polymannose-type oligosaccharides from the endoplasmic reticulum into the cytosol is inhibited by mannosides and requires a thapsigargin-sensitive calcium store. Glycobiology 8, 373–381 (1998).
Iannotti, M. J., Figard, L., Sokac, A. M. & Sifers, R. N. A Golgi-localized mannosidase (MAN1B1) plays a non-enzymatic gatekeeper role in protein biosynthetic quality control. J. Biol. Chem. 289, 11844–11858 (2014).
Moore, S. Oligosaccharide transport: pumping waste from the ER into lysosomes. Trends Cell Biol. 9, 441–446 (1999).
Winchester, B. Lysosomal metabolism of glycoproteins. Glycobiology 15, 1R–15R (2005).
Suzuki, T. Catabolism of N-glycoproteins in mammalian cells: molecular mechanisms and genetic disorders related to the processes. Mol. Asp. Med. 51, 89–103 (2016).
Harada, Y., Masahara-Negishi, Y. & Suzuki, T. Cytosolic-free oligosaccharides are predominantly generated by the degradation of dolichol-linked oligosaccharides in mammalian cells. Glycobiology 25, 1196–1205 (2015).
Tulsiani, D. R. & Touster, O. Substrate specificities of rat kidney lysosomal and cytosolic alpha-D-mannosidases and effects of swainsonine suggest a role of the cytosolic enzyme in glycoprotein catabolism. J. Biol. Chem. 262, 6506–6514 (1987).
Orzalli, M. H. et al. cGAS-mediated stabilization of IFI16 promotes innate signaling during herpes simplex virus infection. Proc. Natl Acad. Sci. USA 10.1073/pnas.1424637112 (2015).
Kapellos, T. S. et al. A novel real time imaging platform to quantify macrophage phagocytosis. Biochem. Pharmacol. 116, 107–119 (2016).
Carroll, E. C. et al. The vaccine adjuvant chitosan promotes cellular immunity via DNA Sensor cGAS-STING-dependent induction of type I interferons. Immunity 44, 597–608 (2016).
Fong, D. et al. Lysosomal rupture induced by structurally distinct chitosans either promotes a type 1 IFN response or activates the inflammasome in macrophages. Biomaterials 129, 127–138 (2017).
Curtis, M. M. et al. The gut commensal bacteroides thetaiotaomicron exacerbates enteric infection through modification of the metabolic landscape. Cell Host Microbe 16, 759–769 (2014).
Cuskin, F. et al. Human gut Bacteroidetes can utilize yeast mannan through a selfish mechanism. Nature 517, 165–169 (2015).
Robb, M. et al. Molecular characterization of N-glycan degradation and transport in Streptococcus pneumoniae and its contribution to virulence. PLOS Pathogens 13, 1–33 (2017).
Gao, N. et al. Mannose-6-phosphate regulates destruction of lipid-linked oligosaccharides. Mol. Biol. Cell 22, 2994–3009 (2011).
Zhu, M. et al. β-Mannosidosis mice: a model for the human lysosomal storage disease. Hum. Mol. Genet. 15, 493–500 (2006).
van Pelt, J. et al. Accumulation of mannosyl-beta(1----4)-N-acetylglucosamine in fibroblasts and leukocytes of patients with a deficiency of beta-mannosidase. Clin. Chim. acta; Int. J. Clin. Chem. 187, 55–60 (1990).
Riise Stensland, H. M. F. et al. Identification of two novel beta-mannosidosis-associated sequence variants: biochemical analysis of beta-mannosidase (MANBA) missense mutations. Mol. Genet. Metab. 94, 476–480 (2008).
Zhu, M. et al. Beta-mannosidosis mice: a model for the human lysosomal storage disease. Hum. Mol. Genet. 15, 493–500 (2006).
Hasan, M. et al. Trex1 regulates lysosomal biogenesis and interferon-independent activation of antiviral genes. Nat. Immunol. 14, 61–71 (2012).
Hirayama, H., Seino, J., Kitajima, T., Jigami, Y. & Suzuki, T. Free oligosaccharides to monitor glycoprotein endoplasmic reticulum-associated degradation in Saccharomyces cerevisiae. J. Biol. Chem. 285, 12390–12404 (2010).
Hossain, T., Hirayama, H., Harada, Y. & Suzuki, T. Lack of the evidence for the enzymatic catabolism of Man1GlcNAc2 in Saccharomyces cerevisiae. Biosci., Biotechnol., Biochem. 80, 1–6 (2015).
Suzuki, T. et al. Dual-gradient high-performance liquid chromatography for identification of cytosolic high-mannose-type free glycans. Anal. Biochem. 381, 224–232 (2008).
We would like to thank Dr. Jennifer Kohler and members of the Yan lab for valuable discussions. This work was supported by the Lupus Research Alliance (N.Y.), the Clark family CRV Research Foundation (N.Y.), the NIH (AR067135 to N.Y., GM038545 to M.A.L.), the Welch Foundation (I-1831 to N.Y.) and NSF-GRFP fellowship (C.F.).
The authors declare no competing interests.
Journal peer review information: Nature Communications thanks the anonymous reviewer(s) for their contribution to the peer review of this work.
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Fermaintt, C.S., Sano, K., Liu, Z. et al. A bioactive mammalian disaccharide associated with autoimmunity activates STING-TBK1-dependent immune response. Nat Commun 10, 2377 (2019). https://doi.org/10.1038/s41467-019-10319-5