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Proteasome inhibition triggers tissue-specific immune responses against different pathogens in C. elegans [1]

['Manish Grover', 'Department Of Life Sciences', 'Imperial College', 'London', 'United Kingdom', 'Spencer S. Gang', 'School Of Biological Sciences', 'University Of California', 'San Diego', 'La Jolla']

Date: 2024-03

Abstract Protein quality control pathways play important roles in resistance against pathogen infection. For example, the conserved transcription factor SKN-1/NRF up-regulates proteostasis capacity after blockade of the proteasome and also promotes resistance against bacterial infection in the nematode Caenorhabditis elegans. SKN-1/NRF has 3 isoforms, and the SKN-1A/NRF1 isoform, in particular, regulates proteasomal gene expression upon proteasome dysfunction as part of a conserved bounce-back response. We report here that, in contrast to the previously reported role of SKN-1 in promoting resistance against bacterial infection, loss-of-function mutants in skn-1a and its activating enzymes ddi-1 and png-1 show constitutive expression of immune response programs against natural eukaryotic pathogens of C. elegans. These programs are the oomycete recognition response (ORR), which promotes resistance against oomycetes that infect through the epidermis, and the intracellular pathogen response (IPR), which promotes resistance against intestine-infecting microsporidia. Consequently, skn-1a mutants show increased resistance to both oomycete and microsporidia infections. We also report that almost all ORR/IPR genes induced in common between these programs are regulated by the proteasome and interestingly, specific ORR/IPR genes can be induced in distinct tissues depending on the exact trigger. Furthermore, we show that increasing proteasome function significantly reduces oomycete-mediated induction of multiple ORR markers. Altogether, our findings demonstrate that proteasome regulation keeps innate immune responses in check in a tissue-specific manner against natural eukaryotic pathogens of the C. elegans epidermis and intestine.

Citation: Grover M, Gang SS, Troemel ER, Barkoulas M (2024) Proteasome inhibition triggers tissue-specific immune responses against different pathogens in C. elegans. PLoS Biol 22(3): e3002543. https://doi.org/10.1371/journal.pbio.3002543 Academic Editor: Hans-Uwe Simon, University of Bern, SWITZERLAND Received: August 23, 2023; Accepted: February 9, 2024; Published: March 11, 2024 Copyright: © 2024 Grover et al. This is an open access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited. Data Availability: All relevant data are within the paper and its Supporting Information files. All RNAseq files are available from the NCBI GEO database (accession number GSE241087). Funding: This work was supported by the Wellcome Trust, UK (219448/Z/19/Z to MB) and the Biotechnology and Biological Sciences Research Council, UK (BB/X001865/1 to MB and ERT). The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript. Competing interests: The authors have declared that no competing interests exist. Abbreviations: BTZ, bortezomib; EMS, ethyl methanesulfonate; IPR, intracellular pathogen response; ORR, oomycete recognition response; PRAAS, proteasome-associated autoinflammatory syndrome; smFISH, single molecule fluorescence in situ hybridization; UPR, unfolded protein response

Introduction The evolutionary history of Caenorhabditis elegans is shaped by various biotic interactions in its natural habitat [1]. These interactions include beneficial and pathogenic microbes, which trigger a diverse set of responses in C. elegans [1]. Studying C. elegans under some conditions encountered in its natural environment can provide novel insights, such as new functions for genes lacking functional annotation in the genome [1]. For example, the identification of oomycetes as natural pathogens of C. elegans revealed a previously uncharacterized family of chitinase-like (chil) genes as immune response effectors, which can modify cuticle properties to prevent oomycete attachment and consequently infection [2]. Most chil genes are not expressed in lab culture conditions and can only be induced upon pathogen recognition together with a broader subset of genes previously described as the oomycete recognition response (ORR) [3]. C. elegans can similarly mount specific responses against other natural pathogens as well, for example, the intracellular pathogen response (IPR) against microsporidia and the Orsay virus [4,5]. While the nematode is likely to use its sensory capabilities to detect pathogens and activate pathogen-specific responses [6], it also uses surveillance immunity as a broad way to tackle pathogenic attacks [7]. Pathogens can hijack the host cellular machinery to support their growth and development, and in doing so, they may disrupt core cellular processes, such as transcription, translation, protein turnover, and mitochondrial respiration. As a result, disruption to these processes can be sensed as a pathogenic attack leading to activation of immune responses [8–10]. For example, inhibition of translation by Pseudomonas aeruginosa exotoxin A leads to activation of immune response genes through transcription factors such as ZIP-2 and CEBP-2 [8,9,11]. Disruption of mitochondrial proteostasis by P. aeruginosa also induces immune responses [12,13]. Similarly, RNAi and microbial toxin perturbation of various core cellular processes induces detoxification enzymes and aversion behavior in C. elegans [10]. Likewise, the IPR can be induced either by inhibition of the purine salvage pathway as seen in pnp-1 mutants [14,15] or by blockade of the major protein degradation machinery in the cell, the proteasome [4,16]. A major player regulating proteostasis upon proteasome blockade is the conserved transcription factor SKN-1/NRF [17,18]. One of its isoforms, SKN-1A (NRF1/NFE2L1 in humans), is normally localized in the endoplasmic reticulum membrane where it is glycosylated and then targeted for proteasomal degradation (Fig 1A) [19]. However, upon proteasome blockade, the glycosylated isoform escapes degradation and is edited by PNG-1 (NGLY1 in humans), a conserved N-glycanase that converts the N-glycosylated asparagine residues to aspartic acid, and the edited protein then translocates to the nucleus [19]. Inside the nucleus, DDI-1 (DDI2 in humans), a conserved aspartic protease, cleaves the N-terminal region of the protein, and this processed SKN-1A is now activated to up-regulate expression of proteasomal subunits to increase proteostasis capacity in a bounce-back response (Fig 1A) [19–21]. In addition to its role in promoting proteostasis capacity, SKN-1 is also required to respond to oxidative stress [22] and promotes resistance to bacterial pathogens, such as the human pathogens P. aeruginosa and Enterococcus faecalis [23–25]. PPT PowerPoint slide

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TIFF original image Download: Fig 1. Proteasome impairment activates ORR in C. elegans. (A) Schematic showing the proteasome surveillance pathway and the stepwise activation of SKN-1A for transcription of proteasomal subunits. (B) L4 stage C. elegans showing constitutive chil-27p::GFP expression in ddi-1(icb156), png-1(icb121), and skn-1a(mg570) mutant animals. Note that skn-1a and png-1 show a stronger, full body activation of the chil-27p::GFP marker in comparison to ddi-1 mutants, which might reflect the fact that png-1 and skn-1a are essential components of the proteasome surveillance pathway, while ddi-1 has been shown to be dispensable [19]. Scale bar is 100 μm. (C) Venn comparisons showing significant overlap between up-regulated genes in the transcriptome of ddi-1(icb156) and skn-1a(mg570) mutant, and BTZ-treated animals with ORR (RF 13.8, p < 6.171e-50 for comparison with ddi-1; RF 13.6, p < 5.518e-101 for comparison with BTZ and RF 36.0, p < 1.249e-59 value for comparison with skn-1a). (D) ddi-1(mg572), png-1(ok1654), and skn-1a(mg570) mutant animals exhibit reduced susceptibility to infection by M. humicola as compared to WT C. elegans (n = 60 per condition, performed in triplicates, p < 0.001 based on log-rank test, a representative graph for one of the 3 replicates is shown). The numerical data for all 3 replicates is available in Supporting information S1 Data. BTZ, bortezomib; ORR, oomycete recognition response. https://doi.org/10.1371/journal.pbio.3002543.g001 Here, we show that, in contrast to previous studies demonstrating a protective role for SKN-1 in promoting resistance against bacterial pathogens, mutants in the SKN-1A-driven proteasome surveillance pathway result in constitutive expression of ORR and IPR and consequently exhibit resistance against infection by oomycetes and microsporidia. Rescue of skn-1a specifically in the epidermis or the intestine was sufficient to restore wild-type levels of infection by oomycetes and microsporidia, respectively. Moreover, we report that the ORR/IPR genes induced in common in these programs, are also regulated through the proteasome and can be induced in distinct tissues depending on the exact trigger. Notably, we show that by increasing proteasome function, there is a partial inhibition of oomycete-mediated induction of ORR markers, suggesting that the response to pathogens may directly involve stabilization of factors normally degraded by the proteasome. Therefore, our findings, together with other studies in flies and mammals [26–29], highlight how proteasome regulation keeps a range of innate immune responses in check in a tissue-specific manner.

Discussion We demonstrate in this study that mutations in the SKN-1A proteasome surveillance pathway in C. elegans activate the ORR and IPR immune responses employed against distinct natural pathogens that infect through the epidermis or colonize the intestine. Our previous work indicated that blockade of the proteasome leads to induction of IPR genes, which are distinct from SKN-1-regulated genes [4,16], but the connection between the SKN-1-regulated pathway and the ORR/IPR was not clear. Here, we show that both loss of SKN-1A, an ER-localized transcription factor, and impairment of proteasome function induce the genes in common to both ORR and IPR. Furthermore, increasing proteasome function through constitutive proteasomal subunit gene expression or hyperactivity of the proteasome partially inhibits oomycete extract-mediated induction of ORR signature genes. Taken together, we hypothesize that some proteasomally regulated factor(s) normally keep the ORR and IPR immune responses in check in the absence of infection, and upon exposure to specific pathogens such factors can be stabilized in the associated tissue triggering the rapid induction of the respective immune programs (Fig 6). A similar phenomenon has been shown to regulate activation of NF-κB in Drosophila, where IMD is proteasomally degraded owing to permanent presence of UbK48 linkages, which are lost upon bacterial infection thereby stabilizing the protein and activating the pathway [26,27]. Likewise, Uba1-mediated proteasomal degradation of IRF3 in Zebrafish keeps activation of IFN signaling and activation of anti-viral immune response in check [44]. While our findings are consistent with a potential direct role for the proteasome in stabilizing factors that may be necessary for ORR/IPR induction, we cannot rule out that the bounce-back response pathway may also act in parallel. Given that the activation of the chil-27p::GFP marker is observed only in late larval stages in skn-1a mutants or with high doses of BTZ in wild-type animals, we speculate that the extent of proteasome dysfunction may determine the level of activation of the immune response programs. Furthermore, SKN-1A has been recently shown to be involved in lipid homeostasis so it is likely to also influence host immunity in more complex ways and beyond its role in the regulation of proteasome function [45]. PPT PowerPoint slide

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TIFF original image Download: Fig 6. Model based on the findings of this study. The model highlights the interplay of SKN-1A-mediated proteasomal gene expression and activation of ORR and IPR in the epidermis and the intestine, respectively. 1. Under normal conditions, proteasomal degradation of unknown positive regulators (denoted as X factor) keeps activation of immune responses in check. 2. When proteasome dysfunction happens either by BTZ treatment or loss-of-function of skn-1a, X-factor escapes degradation and activates ORR and IPR in the epidermis and the intestine. Simultaneously, BTZ-mediated inhibition increases proteasomal gene expression as a bounce-back response. Such X factors could be directly involved in the tissue-specific signaling pathway activated upon oomycete or microsporidia exposure, respectively, in the epidermis and the intestine. Alternatively, they could regulate ORR and IPR gene induction in parallel to the pathogen-induced signaling pathway. BTZ, bortezomib; IPR, intracellular pathogen response; ORR, oomycete recognition response. https://doi.org/10.1371/journal.pbio.3002543.g006 Unwanted activation of immune responses is often accompanied by trade-offs emphasizing the importance of keeping them in check [46]. For example, in pals-22 loss-of-function mutants, constitutive activation of ORR/IPR provides them protection from oomycetes and microsporidia [3]. However, pals-22 mutants also exhibit slow development, reduced lifespan, and increased pathogen load upon exposure to P. aeruginosa [16]. Likewise, pals-17 loss-of-function mutants exhibit constitutive activation of IPR and immunity to intracellular pathogens, but impaired development and reproduction [47]. While skn-1a(mg570) mutants develop normally like wild-type C. elegans, they too exhibit increased age-associated protein aggregation and consequently have a reduced lifespan [34], so similar trade-offs may also come into play in this case and involve proteotoxicity-driven defects that may exacerbate upon stressful conditions. Likewise, human patients with proteasome-associated autoinflammatory syndromes (PRAAS) show hyperactivation of IFN signaling, but often suffer with severe neurodevelopmental anomalies and skeletal defects [28,29,48]. Our study also highlights the importance of isoform-specific functions for skn-1. While skn-1b is neuronally expressed and regulates satiety and metabolic homeostasis [49], skn-1a and skn-1c are likely to have distinct immunomodulatory functions acting in a pathogen-specific way. Previous studies that reported a requirement of skn-1 for bacterial resistance used either skn-1 RNAi or skn-1 mutant alleles that affected both a and c isoforms [24,25]. However, we now show that skn-1a mutants show enhanced resistance to infection by eukaryotic natural pathogens and do not show enhanced susceptibility to PA14, which suggests that bacterial immunity is likely to be driven by SKN-1C or that SKN-1A/C isoforms might have redundant roles in this case. This result also aligns with the fact that just like NRF2 in humans, SKN-1C regulates response to oxidative stress in C. elegans [22], and bacterial pathogens have been shown to trigger ROS production in the host [23]. While proteasome-mediated suppression of inflammatory/immune responses might be an evolutionarily conserved phenomenon, the exact mechanisms of how immune responses are kept in check are likely to differ. For example, activation of type-I interferon signaling in mammals as a consequence of proteasome dysfunction has been attributed to ER stress and activation of the unfolded protein response (UPR) [28,50,51]. This is unlikely to be the case in the context of oomycete recognition as we have previously shown that introducing ER stress does not induce chil-27p::GFP [2]. Similarly, markers of proteotoxic stress are not induced as a part of the ORR/IPR programs, which makes them distinct from other stress-induced responses. Whether proteasomal regulation of the same factors keeps immune responses in check in the C. elegans epidermis and intestine is currently unknown. In the epidermis, the receptor tyrosine kinase OLD-1 is fully required for mounting the ORR and is likely regulated by the proteasome [39]; however, old-1 knockouts are still able to mount the ORR upon skn-1a perturbation ruling out OLD-1 as the main driving factor. In the intestine, ZIP-1 is a plausible candidate because it is degraded by the proteasome under basal conditions and has been shown to be required for induction of a subset of IPR genes [52]. Future work will elucidate the exact proteasomally regulated triggers of ORR/IPR and address whether these are shared or not between different tissues in C. elegans.

Materials and methods C. elegans strains and pathogen maintenance C. elegans strains were cultured on NGM plates seeded with E. coli OP50 at 20°C under standard conditions as previously described [53]. The list of all the strains used in this study is provided in S2 Table. We refer to skn-1(mg570) mutants throughout the manuscript as skn-1a(mg570) to stress that only isoform a is affected. Both M. humicola and N. parisii were maintained as described previously [2,42]. EMS mutagenesis L4 stage WT animals carrying the chil-27p::GFP reporter (icbIs4) were mutagenized with 24 mM ethyl methanesulfonate (EMS) (Sigma) in 4 ml M9, for 4 h with intermittent mixing by inversion. Worm pellets were then washed 10 times with 15 ml M9 to completely get rid of EMS from the suspension and worms were plated onto 90 mm NGM plate seeded with E. coli OP50. After 24 h, 300 adults were randomly picked and divided into thirty 90 mm plates carrying 10 animals in each. After 72 h at 20°C, all F1 gravid adults in each plate were individually bleached and respective pool of F2 embryos were collected onto new plates. Around 60,000 haploid genomes were screened to identify animals showing constitutive activation of chil-27p::GFP. The causative mutations were mapped to ddi-1 and png-1 by crossing to the highly polymorphic CB4856 strain, and 15–25 F2 recombinants were pooled in equal proportion to obtain genomic DNA for whole-genome sequencing of each independent mutant, performed by BGI (Hong Kong). WGS data was analyzed using the CloudMap Hawaiian variant mapping pipeline to identify causative mutations [54]. Oomycete M. humicola infection assays Five M. humicola infected (dead) animals were added to the lawn of E. coli OP50 on 3 NGM plates and 20 live L4 animals for each genotype were transferred individually to each plate (n = 60 per condition per repeat). Dead animals with visible sporangia were scored every 48 h and live animals were transferred to a new NGM plate with 6 M. humicola infected (dead) animals. Dead animals without evidence of infection or animals missing from the plate were censored. Infection assays were performed in triplicates at 20°C on 30 mm NGM plates seeded with 100 μl E. coli OP50. For infection assays upon skn-1 RNAi, embryos were collected by bleaching gravid adults and were grown on E. coli HT115 (control RNAi) or skn-1 RNAi bacteria until the adult stage, which were then used to perform infection assay as described above. Similarly, embryos from WT animals were grown on E. coli OP50 until early L4 stage and then were transferred to OP50 plates with 20 μm of BTZ (Sigma) or DMSO (Thermo Scientific) (control, <0.1%) for 24 h before using them for infection assay. P. aeruginosa PA14 infection assays A total of 100 μl of overnight grown PA14 culture in LB was spread on a 55 mm NGM plate containing 10 μg/ml FuDR. The plates were incubated at 37°C for 24 h, and 90 Day 1 adults grown on NGM-OP50 or NGM-HT115/skn-1 RNAi in the presence of FuDR were transferred to 3 plates each containing 30 animals (in triplicates) and incubated at 25°C. The number of animals alive was counted every 24 h and dead animals defined as unresponsive to touch were removed from the plate. The experiment was continued until all animals on the plate were dead. Microsporidia N. parisii infection assays The 600 synchronized L1 stage worms for each genotype were plated to NGM + E. coli OP50-1 and grown to the young adult life stage at 23°C (48 h for all stains except for pals-22(jy1) mutants, which are developmentally delayed [5] and therefore were grown for 52 h). The 600 young adults were washed off the plate with M9 + 0.1% Tween-20 (M9-T), pelleted, and the supernatant was removed. The worms were then mixed with 2 million N. parisii spores (strain ERTm1), 50 μl of 10× concentrated E. coli OP50-1, and M9 to a final volume of 300 μl. The infection mix was top-plated over the entire surface of a 6-cm NGM plate, dried at room temperature, and transferred to 25°C for 3 h. Following the 3 h pulse infection, the worms were collected from the infection plate with M9-T into a 1.5 ml microcentrifuge tube, pelleted, and then washed 3 additional times with 1 ml of M9-T. The infected worms were then transferred to an NGM + E. coli OP50-1 plate without N. parisii spores and returned to 25°C for an additional 27 h. Infected animals were then fixed in 100% acetone and incubated at 46°C overnight with FISH probes conjugated to the red Cal Fluor 610 fluorophore that hybridize to N. parisii ribosomal RNA (Biosearch Technologies). Samples were analyzed for N. parisii meronts [55] using an ImageXpress Nano plate reader using the 4× objective (Molecular Devices, LLC). The worm area was traced using FIJI software and the average red fluorescence intensity of each worm was quantified with the background fluorescence of the well subtracted, and 50 animals per genotype were quantified for each experimental replicate, and 3 independent infection experiments were performed. For the tissue-specific skn-1a rescue strains MBA1660, MBA1661, and MBA1662, approximately 100 bus-1p::GFP-expressing worms were manually picked onto N. parisii infection assay plates. For consistency, approximately 100 adults for WT and skn-1a(mg570) controls were also picked in the same manner and pulse infection was performed as described above. To remove any potential bias, the order in which strains were picked was randomized from assay to assay, and the 30 hpi endpoints were staggered to account for picking time. Fixation and FISH hybridization were performed as described above. For quantification, fixed animals for each strain were mounted to a 5% agarose pad on a microscope slide and imaged on a Zeiss AxioImager M1 compound microscope using a 2.5× objective. The worm area was traced using FIJI software and the average red fluorescence intensity of each worm was quantified with the background fluorescence of the slide subtracted. In some samples, we observed dim red autofluorescence from embryos inside the adult gonad. Thus, this region of the worm was omitted in all samples when tracing the worm area. Analysis with the ImageXpress plate reader and Zeiss AxioImager produced different arbitrary values for N. parisii FISH pixel intensity. However, the fold difference in infection between WT animals and skn-1a(mg570) mutants was similar (WT animals are approximately 1.5-fold more infected than skn-1a(mg570)) by both imaging and quantification methods, and 50 animals per genotype were quantified for each experimental replicate, and 3 independent infection experiments were performed. RNAseq For transcriptome analysis, synchronized L4 stage animals were collected in triplicates for RNA extraction using TRIzol (Invitrogen) and isopropanol/ethanol precipitation. RNA sequencing was completed by BGI (Hong Kong). Kallisto [56] was used for alignments with the WS283 transcriptome from Wormbase. Count analysis was performed using Sleuth [57] along with a Wald test to calculate log 2 fold changes. All RNAseq data files are publicly available from the NCBI GEO database under the accession number GSE241087. RT-qPCR Synchronized L4 stage animals with 4-h extract treatment or without were collected in TRIzol (Invitrogen) followed by RNA extraction using isopropanol/ethanol precipitation. RNA was quantified using NanoDrop (Thermo Scientific) and its quality was analyzed by gel electrophoresis. cDNA was synthesized using 2 μg RNA with Superscript IV (Invitrogen) and Oligo(dT) primers as per manufacturer’s instructions. Real-time PCR was performed using qPCR primer pairs listed in S2 Table and LightCycler480 SYBR Green I Master Mix (Roche) in a LightCycler480 instrument, and Ct values were derived using the LightCycler480 software and second derivative maximum method. All experiments were performed in biological triplicates and changes in expression were calculated via the 2-ΔΔCt method. Microscopy Animals to be imaged were picked into a drop (5 to 7 μl) of M9 containing sodium azide (50 μm) on an agarose (1%) pad made on a glass slide. Coverslip was added once the animals were paralyzed, and the pad was almost dry. chil-27p::GFP/col-12p::mCherry expression was observed on Zeiss Axio Zoom V16 microscope and images were taken using the associated ZEN Microscopy software. For rpt-3p::GFP and sur-5::UbV-GFP, animals were treated with oomycete extract or 20 μm BTZ with DMSO control for 24 h at early L2 stage and expression was observed on Zeiss Compound microscope (AxioScope A1) at 40× magnification and images were taken using OCULAR. For chil-27p::GFP expression upon BTZ treatment, early L4 stage animals were treated with different doses of BTZ for 24 h and adults were imaged as described above. Molecular cloning and transgenesis To generate constructs for tissue-specific rescue of skn-1a(mg570) mutant, skn-1a fragment was amplified from N2 cDNA using primers skn-1a_fullF and skn-1a_fullR. Promoter fragments, namely, rab-3p and vha-6p were amplified from N2 genomic DNA using primer pairs BJ97-pRab-3Fwd, rab-3rev-skn1, bj97 vha-6 Fwd, and vha-6 Rev skn-1a, respectively. The terminator sequence from 3′UTR of unc-54 was PCR amplified from N2 genomic DNA using primers unc-54-F-skn1a and BJ36_unc-54terR. Plasmids for neuronal and intestinal rescue were assembled with specific promoter, skn-1a and unc-54 3′UTR fragments ligated into SpeI (FastDigest)-digested pBJ97 by Gibson cloning. To make the epidermal rescue plasmid, skn-1a was PCR amplified from N2 cDNA using primers dpy-7_skn-1F and dpy-7_skn-1R and was assembled into PmeI(FastDigest)-digested pIR6 by Gibson cloning. All constructs were individually injected into skn-1a(mg570) at 5 ng/μl with 25 ng/μl of pRJM163 (bus-1p::GFP) as the co-injection marker and 80 ng/μl of pBJ36 as carrier DNA. The transgenic strains thus created were used for microsporidia pathogen load assays. Similarly, all constructs were individually also injected in the strain MBA1055, which is skn-1a(mg570) mutant with chil-27p::GFP reporter in the background. For these injections, 5 ng/μl of rescue plasmid with 5 ng/μl of myo-2p::GFP as co-injection marker and 100 ng/μl of pBJ36 as carrier DNA was used. The transgenic strains thus created were analyzed for expression of chil-27p::GFP in skn-1a(mg570) mutants. RNAi RNAi by feeding was used as the means to induce gene knockdown in C. elegans as previously described [58]. The RNAi clone for skn-1 was obtained from the ORFeome Library (Horizon Discovery) [59] and for wdr-23 and rpt-5 were obtained from the Ahringer Library (Source BioScience) [60]. Both the clones were confirmed by sequencing prior to use. Embryos collected by bleaching gravid adults were added onto NGM plates seeded with E. coli HT115 and contained 1 mM IPTG (Sigma) to induce expression of dsRNA. After 72 h of incubation at 20°C, animals at L4/adult stage were scored for chil-27p::GFP expression (n > 50). The strains used for tissue-specific RNAi were generated by introducing the chil-27p::GFP reporter in previously described strains listed in S2 Table with their associated references. smFISH For inducing the ORR, synchronized L2 stage animals were treated with oomycete extract for 4 h. For inducing IPR, animals were subjected to prolonged heat stress by incubating synchronized L1s at 30°C for 24 h. For causing proteasome dysfunction, synchronized L2 stage animals were treated with 20 μm BTZ treatment for 15 min or 2 h. Following requisite treatment along with relevant controls, animals were fixed with 4% formaldehyde (Sigma-Aldrich) in 1× PBS (Ambion) for 45 min and were permeabilised with 70% ethanol for 24 h. Hybridization was performed at 30°C for 16 h. List of oligos included in all the probes can be found in S2 Table. Imaging was performed in an inverted and fully motorized epifluorescence microscope (Nikon Ti-eclipse) with an iKon M DU-934 CCD camera (Andor) controlled via the NIS-Elements software (Nikon) using the 100× objective. Detailed protocol can be found in [61].

Acknowledgments We thank Domenica Ippolito and Kenneth Liu for comments on the manuscript. Some strains were provided by the CGC, which is funded by NIH Office of Research Infrastructure Programs (P40 OD010440). We thank Gary Ruvkun, Thorsten Hoppe, Keith Choe, and David Smith for strains.

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