An Intricate Network Involving the Argonaute ALG-1 Modulates Organismal Resistance to Oxidative Stress

Carlos A Vergani-Junior; Raíssa De P Moro; Silas Pinto; Evandro A De-Souza; Henrique Camara; Deisi L Braga; Guilherme Tonon-da-Silva; Thiago L Knittel; Gabriel P Ruiz; Raissa G Ludwig; Katlin B Massirer; William B Mair; Marcelo A Mori

doi:10.1038/s41467-024-47306-4

. 2024 Apr 9;15:3070. doi: 10.1038/s41467-024-47306-4

An Intricate Network Involving the Argonaute ALG-1 Modulates Organismal Resistance to Oxidative Stress

Carlos A Vergani-Junior ^1,^2,^#, Raíssa De P Moro ^1,^2,^#, Silas Pinto ^1,², Evandro A De-Souza ¹, Henrique Camara ^1,^2,³, Deisi L Braga ^1,², Guilherme Tonon-da-Silva ^1,², Thiago L Knittel ^1,², Gabriel P Ruiz ^1,², Raissa G Ludwig ^1,², Katlin B Massirer ^4,⁵, William B Mair ⁶, Marcelo A Mori ^1,^2,^7,^8,^✉

PMCID: PMC11003958 PMID: 38594249

Abstract

Cellular response to redox imbalance is crucial for organismal health. microRNAs are implicated in stress responses. ALG-1, the C. elegans ortholog of human AGO2, plays an essential role in microRNA processing and function. Here we investigated the mechanisms governing ALG-1 expression in C. elegans and the players controlling lifespan and stress resistance downstream of ALG-1. We show that upregulation of ALG-1 is a shared feature in conditions linked to increased longevity (e.g., germline-deficient glp-1 mutants). ALG-1 knockdown reduces lifespan and oxidative stress resistance, while overexpression enhances survival against pro-oxidant agents but not heat or reductive stress. R02D3.7 represses alg-1 expression, impacting oxidative stress resistance at least in part via ALG-1. microRNAs upregulated in glp-1 mutants (miR-87-3p, miR-230-3p, and miR-235-3p) can target genes in the protein disulfide isomerase pathway and protect against oxidative stress. This study unveils a tightly regulated network involving transcription factors and microRNAs which controls organisms’ ability to withstand oxidative stress.

Subject terms: Gene regulation, miRNAs, Ageing

In this study, Vergani-Junior et al. show that increased expression of the argonaute ALG-1 in long-lived worms improves oxidative stress resistance through the modulation of microRNAs that downregulate the protein disulfide isomerase pathway.

Introduction

Aging is associated with the decreased ability of cells to respond to endogenous and exogenous stressors^1,2. This impaired response to stressful perturbations results in surplus of toxic products, such as reactive oxygen species (ROS), thus impairing health². Caenorhabditis elegans is a widely used model organism in aging research and has been fundamental for the identification and characterization of mechanisms involved in life and health span regulation^1,3,4.

One of such mechanisms involve microRNAs (miRNAs) – small non-coding RNAs known to operate by targeting mRNAs through base complementarity and fine-tuning gene expression by inhibiting translation and/or promoting mRNA decay⁵. Since the identification of lin-4 as a miRNA involved in longevity in C. elegans⁶, other miRNAs have been found to modulate stress responses and the aging process across the evolutionary spectrum^5,7. For instance, genetic loss of mir-71 shortens the lifespan of C. elegans, whereas overexpression of this miRNA promotes longevity through pathways involving the transcription factor DAF-16, the worm ortholog of FoxO^8,9. In addition, mir-71 mutants fail to properly regulate proteostasis¹⁰.

Pathways that lead to longevity have been shown to involve at least in part mechanisms that enable organisms to deal more efficiently with stress. For instance, germline deficiency caused by mutation of the C. elegans Notch ortholog glp-1 results in extended lifespan and improved oxidative stress response^11–13. Interestingly, lifespan extension promoted by the glp-1 mutation depends on both DAF-16/FoxO and miR-71⁹. The mechanism through which germline deficiency protects from oxidative stress at the organismal level is less understood.

The C. elegans argonaute ALG-1 (Ago-like gene 1), like its human ortholog AGO2, is an endoribonuclease that plays a fundamental role in miRNA processing and function¹⁴. ALG-1 assembles and stabilizes guide strands from miRNA duplexes, pairing them with target mRNAs, thereby mediating target degradation or repression¹⁴. Inhibition of ALG-1 disrupts miRNA function and leads to a global reduction of mature miRNAs in the worm and accumulation of pre-miRNAs^15,16. In C. elegans, the expression of alg-1 decreases with aging, and alg-1 loss-of-function results in developmental defects, as well as decreased oocyte number, shorter lifespan, and increased stress sensitivity^14,16–18. ALG-1 is also required for proper heat stress recovery response¹⁹. Although there is mounting evidence showing how miRNAs and argonautes participate in multiple biological processes, including aging, whether these enzymes can be physiologically regulated to modify the ability of organisms to respond to environmental perturbations and adapt to stress remains to be elucidated.

Here we show in C. elegans that ALG-1 upregulation is a common feature among a number of conditions leading to extended lifespan. Knockdown of alg-1 in adult worms reduces lifespan, impairs resistance to pro-oxidant agents, and suppresses the increased longevity and oxidative stress resistance of germline-deficient glp-1 mutants. In contrast, worms overexpressing alg-1 are protected from oxidative stress, but not from heat or reductive stress. We identified R02D3.7 as a repressor of alg-1 and showed it to be downregulated in glp-1 mutants and involved in oxidative stress resistance. We also explored the downstream mechanisms through which ALG-1 modulates stress resistance, and found miRNAs upregulated in glp-1 mutants (i.e., miR-87-3p, miR-230-3p, and miR-235-3p) involved in oxidative stress response. Genes associated with the protein disulfide isomerase (PDI) pathway are enriched among the putative targets of these miRNAs, and we showed that miR-230-3p can directly target pdi-2 - the ortholog of the human gene encoding protein disulfide isomerase P4HB. Moreover, partial reduction of pdi-2 results in increased survival when worms are exposed to paraquat – a pro-oxidant agent. Taking these results together, we conclude that upregulation of the argonaute ALG-1 represents a mechanism that helps worms resist oxidative stress by increasing the activity of miRNAs that can target the PDI pathway.

Results

Loss of alg-1 in adult C. elegans disrupts redox balance

Deficiency in alg-1 has a broad range of effects in C. elegans, some of which are developmental, i.e., occurring prior to adulthood^15,20. The levels of ALG-1 reduce with aging^17,21 and alg-1 deficiency shortens lifespan^17,22. When alg-1 RNAi is applied during adulthood to dissociate from its developmental effects, this intervention also reduces lifespan (Supplementary Fig. 1a). While the phenotype of reduced lifespan has been consistently confirmed by other studies^17,22, the mechanisms through which ALG-1 regulates worm vitality and stress resistance remain unclear.

Consistent with an impaired oxidative stress response in alg-1 deficient worms¹⁸, we found increased mortality in alg-1 RNAi vs. control RNAi (empty vector) when subjecting worms to pro-oxidant agent paraquat (Supplementary Fig. 1b). alg-1 RNAi also increased superoxide dismutase 3 (sod-3) (Supplementary Fig. 1c) and glutathione S-transferase 4 (gst-4) (Supplementary Fig. 1d) promoter activities – known to be induced by oxidative stress. The level of induction of the sod-3 and gst-4 transcriptional reporters by alg-1 RNAi was equivalent to that induced by paraquat. Moreover, paraquat did not further increase the levels of sod-3p::GFP in worms treated with alg-1 RNAi. These results demonstrate that ALG-1 is necessary in adult worms for proper control of redox homeostasis and oxidative stress resistance.

ALG-1 is upregulated in multiple long-lived mutants

Given the role of ALG-1 in lifespan and redox homeostasis, we questioned whether alg-1 expression was increased in long-lived mutants. By analyzing RNA sequencing (RNAseq) data from long-lived worms (GSE111338 from Gene Expression Omnibus and Dutta, et al.²³), we observed that alg-1 mRNA was upregulated in the germline-deficient mutant glp-1(e2141), the electron transport chain-deficient mutant clk-1(qm30), the dietary-restricted mutant eat-2(ad1116), and the mTORC1-deficient mutant raga-1(ok386), but not in the insulin/IGF1 signaling-deficient mutant age-1(hx546) (Fig. 1a and Supplementary Data 1). On the other hand, alg-2 - a paralog of alg-1 also involved in miRNA function¹⁶ - was not affected in these long-lived mutants, except for the eat-2 mutant, where alg-2 was increased, and the glp-1(e2141) mutant, where alg-2 was downregulated (Supplementary Fig. 2a).

Fig. 1 — a *alg-1* gene expression in long-lived mutants as determined by RNAseq. n = 4 per group. Values represent log₂(fold change of long-lived mutant/control), logFC. Adjusted P values and detailed information are described in Supplementary Data 1. b Representative images and c relative GFP fluorescence of the *gfp::alg-1* reporter (PQ530) in different long-lived mutant backgrounds at day 1 of adulthood. Combined data of two independent replicates. n = 20, 20, 18, 18, 22 worms per condition. d Schematic of the RNAi screen used to find and validate *alg-1* regulators. Two *gfp::alg-1* reporter strains were used, CT20²⁵, a multicopy integrated *alg-1p::gfp::alg-*1 transgene (*zals5*) and, PQ530¹⁷, a endogenous *alg-1* allele (*ap423*) tagged with GFP. Created with BioRender.com. Relative GFP fluorescence of CT20 (n = 30, 27, 33, 31, 31, 28, 26 worms per condition) (e) and PQ530 (n = 32, 29, 31, 28, 28, 35, 36 worms per condition) (f) worms after RNAi exposure. Worms were grown on plates with control (ctrl) RNAi (empty vector), transferred to respective RNAi plates at day 0 of adulthood, and had their fluorescence measured on day 3. Combined data of three independent experiments. g *gei-2/mep-1, nhr-28, nhr-77, R02D3.7* and *skn-1* gene expression in long-lived mutants as determined by RNAseq. n = 4 per group. * Adjusted P values < 0.05, as described on Supplementary Data 1. c, e, f Bars represent mean ± SEM. Comparisons between controls groups *versus* experimental groups were made using one-way ANOVA with Dunnett’s post hoc test. ns – non-significant (P > 0.05), * P < 0.05, **P < 0.01, ***P < 0.001, ****P < 0.0001. Source data and exact P values (whenever available) are provided in the Source Data file.

For that reason, and because the role of ALG-2 in longevity and stress resistance remains contentious^17,18, in this study we decided to focus on ALG-1. Using a CRISPR-engineered ALG-1 reporter strain generated by the Pasquinelli group where GFP was fused to the N-terminus of endogenous ALG-1¹⁷ (PQ530), we confirmed that the upregulation of ALG-1 occurred at the protein level in all mutants where alg-1 mRNA was upregulated (Fig. 1b, c). The glp-1(e2144) mutant exhibited the highest ALG-1 expression among the long-lived mutants. Thus, we used glp-1(e2144) mutants for the remainder of the study to better comprehend ALG-1 regulation and its association with stress resistance in a condition of extended longevity.

To understand how ALG-1 expression can be transcriptionally controlled and dynamically regulated, we searched for transcription factors that bind to the alg-1 promoter and control its expression. Using the modENCODE project - a validated ChIP-Seq database of C. elegans²⁴ - we found 24 transcription factors capable of binding to a 2-kb element upstream of the alg-1 starting codon (Fig. 1d and Supplementary Data 2). First, we tested the ability of these transcription factors to control ALG-1 levels using an RNAi screen employing a multicopy, integrated alg-1p::gfp::alg-1 transgenic reporter strain generated by Shih-Peng Chan & Frank Slack (CT20)²⁵.

Of the 24 candidates, knockdown of 5 of them (gei-2/mep-1, nhr-28, nhr-77, R02D3.7, and skn-1) increased the levels of ALG-1 (Fig. 1e). To further validate these candidates as regulators of alg-1, we used the CRISPR-engineered ALG-1 reporter strain PQ530. In PQ530 worms, ALG-1 levels increased following the knockdown of gei-2, nhr-77, or R02D3.7, with no changes observed under nhr-28 and skn-1 RNAi (Fig. 1f). These results confirm GEI-2, NHR-77, and R02D3.7 as negative regulators of ALG-1.

We then investigated the expression levels of gei-2, nhr-77, and R02D3.7 in the RNAseq datasets of long-lived mutants. We found that R02D3.7 was downregulated in all long-lived mutants where alg-1 was upregulated (Fig. 1g), agreeing with its role as a negative regulator of alg-1. The pattern of gei-2 was less consistent, whereas it was also downregulated in glp-1(2144) mutants. In contrast, nhr-77 was not altered in the long-lived mutants (Fig. 1g and Supplementary Data 1). Knockdown of R02D3.7, but not gei-2, further increased ALG-1 expression in glp-1(e2144) mutants (Supplementary Fig. 2b), although to a lesser magnitude than in wild type (WT) worms (Fig. 1e). Together, these results identify three genes that exert negative regulation over alg-1; two of them, namely R02D3.7 and gei-2, are associated with the upregulation of ALG-1 in long-lived mutants.

While the binding of these transcription factors to the alg-1 promoter suggests their cis-regulatory role in controlling alg-1 transcription, the verification of their functionality in a screen utilizing reporter strains where the alg-1 promoter governs the expression of GFP::ALG-1 fusion proteins potentially influenced by the endogenous 5’ and 3’ UTRs does not preclude the possibility of their acting in trans. For instance, they might exert an indirect influence through the induction of miRNAs that suppress ALG-1 expression. Indeed, the long-lived phenotype of glp-1 mutants depends on miR-71⁹, which is itself a negative regulator of ALG-1²¹. Hence, the reduction of a positive regulator of miR-71 could explain the upregulation of ALG-1.

In agreement with this possibility, a null mutation in the mir-71 gene upregulated ALG-1 in the ALG-1 reporter strain CT20 (Supplementary Fig. 2c). We then tested if gei-2 and R02D3.7, which are downregulated in glp-1 mutants and suppress ALG-1 levels, control the activity of the mir-71 promoter (Supplementary Fig. 2d). Only the knockdown of gei-2 influenced mir-71 promoter activity, resulting in downregulation. Consistent with a function of GEI-2 suppressing ALG-1 via induction of miR-71, gei-2 RNAi did not induce GFP::ALG-1 levels in mir-71 mutant worms (Supplementary Fig. 2e). These findings unveil a complex regulatory network governing ALG-1 levels, wherein transcription factors can modulate ALG-1 expression both in cis through direct promoter binding and in trans by inducing miRNAs that negatively regulate its mRNA.

Worms overexpressing ALG-1 are oxidative stress resistant

To investigate whether upregulation of ALG-1 is sufficient to prolong worm lifespan and protect adult worms from stress, we studied worms overexpressing alg-1 (ALG-1/OE) (Supplementary Fig. 3a–d). One of these models carries a multicopy transgene inserted in the genome from which a GFP::ALG-1 fusion functional protein is overexpressed (CT20)²⁵ – the same model used as one of the ALG-1 reporter strains in the previous experiments (Fig. 1d). In this case, to control for the transgene expression, we compared these worms to worms carrying a transgene overexpressing a luciferase::GFP fusion protein (PE255), a strain generated by Cristina Lagido²⁶, which we have denoted as the ctrl strain.

We also made use of another ALG-1/OE model, in which the 3’UTR of alg-1 was substituted by the Y45F10D.4 3’UTR using CRISPR/Cas9 editing (PQ535), thus avoiding the negative regulation exerted by miRNAs, as designed, and previously reported by the Pasquinelli lab¹⁷. In this case, we used the WT as the control. Both models exhibited at least 4-fold increases in alg-1 mRNA levels in comparison to their respective controls (Supplementary Fig. 3b and d).

While none of the ALG-1/OE strains lived longer or had a consistent delay in the progression of age-related features such as the decline in mobility and pharyngeal pumping capacity (Supplementary Fig. 4a–f), the PQ535 strain exhibited delayed duration of development (Supplementary Fig. 4g) and reduced brood size (Supplementary Fig. 4h) when compared to WT worms, in agreement with the crucial role of miRNAs in development and reproduction^27–29.

However, bacterial-derived nitric oxide (NO), a free radical known to inhibit ALG-1 post-translationally³⁰ and to play a role in worm redox reactions and signaling pathways^31–34, influences ALG-1/OE effects on C. elegans lifespan, as worms overexpressing ALG-1 lived longer than controls when fed with B. subtilis (∆NOS) that do not produce NO (Supplementary Fig. 4i). In contrast, and like E. coli, in the presence of wild type B. subtilis ALG-1/OE worms lived as long as the controls. These phenotypes can be attributed to a decrease in lifespan observed when worms are exposed to bacteria lacking NO, whereas ALG-1 overexpression confers protection against this lifespan reduction. Noteworthy, NO reacts with superoxide to produce peroxynitrite, and in NO deficient conditions, increased superoxide levels and an overreliance on superoxide dismutases to maintain redox balance can be anticipated³⁵.

In agreement with a protective role of ALG-1 overexpression under oxidative stress conditions, ALG-1/OE worms displayed increased resistance against sodium arsenite and paraquat stresses, regardless of the model to overexpress ALG-1 (Fig. 2a–d). Both chemicals are known to enhance superoxide levels, albeit through different mechanisms^36–38. To control for a potential unspecific effect of GFP overexpression, we silenced GFP in the ALG-1/OE (CT20) model and this completely reversed the paraquat resistance phenotype of these worms, consistent with the silencing of the transgene-driven GFP::ALG-1 fusion protein. In contrast, silencing GFP did not affect paraquat sensitivity in the control PE255 strain, which overexpresses the luciferase::GFP fusion protein (Supplementary Fig. 5a).

Germline-deficient glp-1 mutant worms were also more resistant to sodium arsenite and paraquat (Fig. 2e, f), although in the arsenite assay the differences did not reach statistical significance (P = 0.0576 at 15 mM). Furthermore, increased paraquat resistance and longevity of glp-1 mutants required ALG-1 (Fig. 2f and Supplementary Fig. 5b). These findings support the notion that elevated levels of ALG-1 in glp-1 mutants contribute to enhanced resistance against oxidative stress, and further establish the indispensability of ALG-1 for the prolonged survival of germline-deficient worms in both normal and stressful environmental conditions.

The transcription factors DAF-16 and SKN-1 play a role in multiple stress pathways and are required for stress resistance and longevity induced by germline deficiency^13,39–41. This prompted us to investigate whether ALG-1 acted in concert with DAF-16 and SKN-1 to promote oxidative stress resistance. While RNAi targeting daf-16 or skn-1 reduced worm survival under paraquat, ALG-1 overexpression increased worm survival regardless whether daf-16 and skn-1 were knocked down or not (Supplementary Fig. 5c, d), indicating that ALG-1 induction promotes oxidative stress resistance despite the silencing of these transcription factors.

To further explore how ALG-1 upregulation protects from oxidative stress, we evaluated the promoter activity of genes encoding two enzymes involved in antioxidant and detoxification responses – SOD-3 and GST-4. Improved oxidative stress resistance in ALG-1/OE worms accompanied higher sod-3 promoter activity levels at baseline (Fig. 2g), but not gst-4 (Fig. 2h). Paraquat induced sod-3p::GFP and gst-4p::GFP levels in both ALG-1/OE and WT worms, whereas the activity of the sod-3 reporter was higher in ALG-1/OE under this oxidative stress condition (Fig. 2g, h).

The administration of the antioxidant N-acetylcysteine (NAC) blunted the induction of the sod-3 reporter by alg-1 RNAi, but had no impact on WT or ALG-1/OE worms (Fig. 2i). Hence, ALG-1/OE worms remained with higher levels of the sod-3 reporter in comparison to WT worms regardless of the presence of NAC. This suggests that, in contrast with alg-1 knockdown where both sod-3 and gst-4 promoters are induced due to a chronic state of oxidative stress, overexpression of ALG-1 selectively induces sod-3 transcription, thus helping worms to resist superoxide exposure in a preventive manner.

Importantly, the increased stress resistance promoted by ALG-1 overexpression was specific to oxidative stress, given that ALG-1/OE worms were less resistant to dithiothreitol (DTT) - a reducing agent known to induce endoplasmic reticulum (ER) stress^42,43 (Supplementary Fig. 5e) – and as resistant as the controls to heat stress (Supplementary Fig. 5f). Overall, these results show that ALG-1 overexpression is sufficient to enhance worm survival under conditions of oxidative stress.

Downregulation of R02D3.7 protects from oxidative stress

Next, we investigated if the two negative regulators of ALG-1 that are downregulated in glp-1 mutants (i.e., R02D3.7 and gei-2) control oxidative stress response in a manner that involved ALG-1. While R02D3.7 RNAi protected worms from sodium arsenite and paraquat-induced mortality, the knockdown of gei-2 had no significant effect on oxidative stress resistance (Fig. 3a, b). Adding alg-1 RNAi to the R02D3.7 RNAi fully suppressed the effect of R02D3.7 silencing on arsenite stress (Fig. 3c). However, R02D3.7 RNAi could still increase protection from paraquat stress when alg-1 was knocked down, whereas the addition of alg-1 RNAi decreased paraquat resistance when R02D3.7 was silenced (Fig. 3d).

Fig. 3 — a Survival after 8 hours of sodium arsenite exposure on day 3 adults. WT worms were treated with control (empty vector), *gei-2* or *R02D3.7* RNAi since day 0. n = 18, 17, 12, 18, 16, 14 wells with 10 worms each per condition. b Survival on paraquat (8 mM) of WT worms treated with control (empty vector), *gei-2* or *R02D3.7* RNAi since day 0 of adulthood. n = 98 worms for ctrl RNAi; 113 worms for *gei-2* RNAi; 112 worms for *R02D3.7* RNAi. c Survival after 8 hours of sodium arsenite exposure on day 3 adults. WT worms were treated with control (empty vector), *R02D3*.7, *R02D3.7 + alg-1* or *alg-1* RNAi since day 0. n = 18 wells with 10 worms each per condition. d Survival on paraquat (8 mM) of WT worms treated with control (empty vector), *R02D3.7*, *R02D3.7 + alg-1* or *alg-1* RNAi since day 0 of adulthood. n = 91 worms for ctrl RNAi; 99 worms for *alg-1* RNAi; 117 worms for *R02D3.7* RNAi; 78 worms for *R02D3.7+alg-1* RNAi. e Survival on paraquat (8 mM) of WT and ALG-1/OE (PQ535) worms treated with control (empty vector) or *R02D3.7* RNAi since day 0 of adulthood. n = 152 worms for WT ctrl RNAi; 133 worms for WT *R02D3.7* RNAi; 124 worms for ALG-1/OE ctrl RNAi; 118 worms for ALG-1/OE *R02D3.7* RNAi. f Lifespan under normal conditions of WT worms treated with control (empty vector), *R02D3.7*, *R02D3.7 + alg-1* or *alg-1* RNAi since day 0 of adulthood. n = 136 worms for ctrl RNAi; 132 worms for *alg-1* RNAi; 127 worms for *R02D3.7* RNAi; 135 worms for *R02D3.7+alg-1* RNAi. a, c Bars represent mean ± SEM. Combined data of three independent replicates. Comparisons were made using two-way ANOVA with Sidak’s post hoc test. ns – non-significant (P > 0.05), *P < 0.05, ****P < 0.0001. b, **d–f** Representative data from three independent replicates. Data were compared using the log-rank test. ns – non-significant (P > 0.05), *P < 0.05, ***P < 0.001, ****P < 0.0001. Source data and exact P values (whenever available) are provided as a Source Data file.

Furthermore, in contrast to the observed effects on WT worms, the knockdown of R02D3.7 showed limited impact on ALG-1/OE worms, failing to further increase resistance to paraquat (Fig. 3e). Consistent with the normal lifespan of ALG-1/OE worms, R02D3.7 knockdown did not affect survival under unstressed conditions (Fig. 3f). Together, these results show that the downregulation of R02D3.7, which allows higher levels of ALG-1, protects worms from oxidative stress. This phenotype occurs at least partially via ALG-1 and can be mimicked by ALG-1 overexpression.

miRNAs induced by ALG-1/OE confer oxidative stress resistance

We then searched for miRNAs that conferred improved oxidative stress resistance to worms overexpressing ALG-1. Since miR-71 is required for germline deficiency-induced longevity⁹, we first investigated whether miR-71 deficiency interfered with the stress resistance of ALG-1/OE worms. Loss of mir-71 blunted the protection against paraquat (Supplementary Fig. 6a) and sodium arsenite (Supplementary Fig. 6b) promoted by ALG-1/OE, although it did not interfere with oxidative stress resistance of control worms (Supplementary Fig. 6c, d). These results indicate that in addition to being a negative regulator of ALG-1²¹, miR-71 also acts downstream of ALG-1 overexpression to confer increased oxidative stress resistance.

Next, we took an unbiased approach and performed small RNAseq to identify potential miRNAs commonly upregulated in glp-1(e2144) mutants and ALG-1/OE (CT20) worms. Consistent with increased ALG-1 levels in both models, we saw an overall increase in miRNA abundance and a significant overlap (P < 0.02) between the miRNAs upregulated in the two conditions (Fig. 4a–d and Supplementary Data 3). There were 72 miRNAs upregulated in glp-1(e2144) mutants and 36 in ALG-1/OE (CT20) (log₂ fold change > 1), among which 11 were in common (Fig. 4c, e). In contrast, only 22 miRNAs were downregulated in glp-1(e2144) mutants and 4 in ALG-1/OE (CT20) (log₂ fold change < −1), with no overlap (Fig. 4d). Although miR-71 did not fall within the miRNAs affected by ALG-1 overexpression according to our cutoff, it appeared increased in glp-1(e2144).

Fig. 4 — Heatmaps of differentially expressed miRNAs (log₂ fold change > 1 or < −1) on a *glp-1(e2144)* mutants in comparison with WT worms, and b ALG-1/OE (CT20) strain in comparison with its control (ctrl) strain. Detailed information in Supplementary Data 3. Venn diagrams representing the miRNAs (c) upregulated or (d) downregulated on *glp-1(e2144)*, ALG-1/OE (CT20), and in both. e Eleven miRNAs upregulated in both *glp-1(e2144)* mutants and ALG-1/OE worms. f Survival of *mir-235(n4504)* and WT worms after 8 hours of exposure to sodium arsenite on day 3 of adulthood. n = 22, 17, 24, 18 wells with 10 worms each per condition. Bars represent mean ± SEM. Combined data of three independent replicates. Comparisons were made using two-way ANOVA with Sidak’s post hoc test. **P < 0.01, ****P < 0.0001. g–i Survival on paraquat (4 mM) of *mir-87(n4104), mir-230(n4535*) or *mir-235(n4504)* mutants vs. WT. Experiments were performed together and share the same controls, which were split in different panels to allow better visualization. n = 119 worms for WT; 133 worms for *mir-87*; 110 worms for *mir-230*; 123 worms for *mir-235*. Data were compared using the log-rank test. *P < 0.05, ***P < 0.001, ****P < 0.0001. f–i Data represent one experiment of three independent replicates. Source data are provided as a Source Data file.

Of the 11 upregulated miRNAs identified in glp-1(e2144) mutants and ALG-1/OE (CT20) worms, both the 5p and 3p strands of miR-87 and miR-230 were observed, contributing to a total of 9 potential miRNA genes associated with stress resistance (Fig. 4e). Among those, we had access to null mutants of 8 of them (i.e., mir-45, mir-47, mir-87, mir-229, mir-230, mir-235, mir-259, mir-357). Initially, we tested if these mutants were more sensitive to oxidative stress. mir-235 deficiency impaired both arsenite and paraquat stress resistance (Fig. 4f, i), while loss of mir-230 or mir-87 impaired only paraquat-induced mortality (Fig. 4g, h).

Loss of mir-229, on the other hand, improved paraquat stress resistance (Supplementary Fig. 7j). The null mutants for the remaining miRNAs did not show any differences in the resistance to oxidative stress (Supplementary Fig. 7a–l). Loss-of-function mutations in mir-87, mir-230, or mir-235 also led to reduced oxidative stress resistance in ALG-1/OE worms (Supplementary Fig. 8a–f). These findings unveiled miRNAs upregulated in glp-1 mutants and ALG-1/OE worms that take part in regulation of oxidative stress resistance.

miRNAs induced by ALG-1/OE target and limit the PDI pathway

miR-235, miR-230, and miR-87 were the miRNAs that consistently conferred protection against oxidative stress-induced mortality according to our data. Hence, we decided to look for targets of these miRNAs that participate in oxidative stress resistance. We intersected the information of putative targets of these miRNAs (we used target predictions of the 3p strands as it was the information available on the TargetScanWorm database⁴⁴) with possible miRNA targets, i.e., genes found to be upregulated in publicly available microarray data obtained from the alg-1 loss of function mutant alg-1(gk214)⁴⁵ (Fig. 5a).

Fig. 5 — a Schematic of the strategy used to find putative targets of the miRNAs upregulated in response to *alg-1* overexpression and involved in oxidative stress resistance. b Approach used to validate *pdi-*2 as a target of miR-230-3p. Cel-miR-230-3p or cel-miR-85-3p (negative control) mimics were administrated in HEK293T cells transfected with luciferase reporter vectors containing the *pdi-2* 3’UTR (native or mutated – Firefly luciferase) or not (Renilla luciferase). Created with BioRender.com c Luminescence ratio of Firefly luciferase (potentially regulated by the presence of *pdi-2* 3’UTR) and Renilla luciferase (transfection control) of HEK293T cells. n = 12 independent cell pools per condition. d Survival of *pdi-2(tm689)* heterozygous (het) mutants and WT worms on paraquat (4 mM). n = 122 for WT and 85 for *pdi-2(tm689)*. e Survival of *pdi-2(tm689)* heterozygous (het) mutants and WT worms after 8 hours of exposure to sodium arsenite on day 3 of adulthood. n = 22, 22, 28, 28 wells with 10 worms each per condition. f Survival on paraquat (8 mM) of WT worms exposed to control (ctrl, empty vector) or *alg-1* RNAi since eggs. n = 91 worms for ctrl RNAi and 131 worms for *pdi-2* RNAi. g Survival after 8 hours of exposure to sodium arsenite on day 3 of adulthood of WT worms exposed to ctrl (empty vector) or *pdi-2* RNAi since eggs. n = 16, 16, 20, 20 wells with 10 worms each per condition. h Lifespan of WT worms exposed to ctrl (empty vector) or *alg-1* RNAi since eggs. n = 142 worms for ctrl RNAi and 146 worms for *pdi-2* RNAi. c, e, g Bars represent mean ± SEM. Combined data from two independent experiments. Comparisons were made using two-way ANOVA with Sidak’s post hoc test. ns – non-significant (P > 0.05), ****P < 0.0001. d, f and h Data were compared using the log-rank test. ****P < 0.0001. Representative data from three independent experiments. Source data and exact P values (whenever available) are provided as a Source Data file.

Out of the 581 genes upregulated in alg-1(gk214) mutants, 41 (7%, P = 7.33e-05) overlapped with 344 putative targets of miR-87-3p, whereas for miR-230-3p and miR-235-3p, there was an overlap of 137 (23.5%, P = 6.32e-60) and 36 (6%, P = 8.07e-07) genes of a total of 1,022 and 223 putative targets, respectively (Supplementary Fig. 9a and Supplementary Data 4). According to the GO Molecular Function database, available at WormEnrichR⁴⁶, these overlapped genes are predicted to have their molecular function associated with the PDI pathway (Supplementary Fig. 9b).

Based on this data, we hypothesized that miRNA-mediated targeting of the PDI pathway could help worms to better resist oxidative stress. Considering that the mRNA of one of the C. elegans PDI isoforms, PDI-2, appeared as a putative direct target of miR-230-3p (Supplementary Data 4), we attempted to confirm this mechanism using a reductionist experimental setting. We transfected HEK293T cells with luciferase reporter vectors carrying the pdi-2 3’UTR (native or mutated) and added the C. elegans miR-230-3p mimic (Fig. 5b). The miR-230-3p mimic inhibited luciferase activity in cells transfected with the vector containing the native pdi-2 3’UTR, but not in cells transfected with the mutated vector (Fig. 5c), confirming that pdi-2 can indeed be a direct target of miR-230-3p.

Furthermore, the partial inhibition of pdi-2 in the pdi-2(tm689) heterozygous loss-of-function mutant protects worms from paraquat or sodium arsenite exposure (Fig. 5d, e). Concordantly, using RNAi to downregulate pdi-2 increased paraquat resistance (Fig. 5f). On the other hand, this approach sensitized worms to sodium arsenite stress (Fig. 5g) and reduced lifespan under normal conditions (Fig. 5h). Taken together, our results demonstrate that upregulation of ALG-1, which occurs in multiple long-lived mutants, enhances oxidative stress resistance by upregulating miRNAs that can target and fine-tune the PDI pathway (Fig. 6).

Fig. 6 — Arrows represent activation. Blunt-end represents inhibition. Continuous lines represent direct regulation. Dashed lines represent indirect regulation. Created with BioRender.com.

Discussion

Aging progressively decreases the ability of cells to respond to stressors. Hence, being able to maintain stress response mechanisms can prolong the general health span of the organism^1,2. Several individual miRNAs participate in pathways directly involved in aging and stress responses^5,7. In the current study, we described a central pathway through which C. elegans modulates the miRNA processing machinery to resist oxidative stress.

We used C. elegans as a model to characterize this pathway since the miRNA processing machinery is highly conserved from nematodes to humans, and mechanisms involved in organismal stress responses and aging are well established in C. elegans and can be more easily assessed in this species. In addition, age-associated changes in components of the miRNA processing machinery such as Dicer and argonautes have been demonstrated in C. elegans and confirmed in vertebrates^17,47. While upregulation of Dicer in C. elegans renders worms stress resistant⁴⁷, studies in multiple organisms suggest that the levels of argonautes are usually limiting when it comes to availability of most miRNAs^16,48. Indeed, argonaute loading has been recently confirmed to represent a key bottleneck for miRNA stabilization⁴⁹. Moreover, Dicer processes different small RNA species, while argonautes such as human AGO2 and C. elegans ALG-1 are specific to miRNA¹⁴. Hence, targeting argonautes may represent a more specific and efficacious way to alter miRNA activity.

While ALG-2, along with ALG-1, contributes to miRNA function and biogenesis in C. elegans, its role in lifespan regulation and stress resistance is less clear. Reductions in lifespan and in stress resistance in alg-1 loss-of-function mutants have been confirmed by different groups, whereas alg-2 loss-of-function mutants have been reported as long-lived or short-lived in different studies^17,18. Moreover, alg-1 loss-of-function mutants are more sensitive to oxidative stress than alg-2 loss-of-function mutants¹⁸. In addition, our findings indicate that while alg-1 levels are induced in several long-lived strains, the levels of alg-2 are not consistently related to longevity in these models.

In line with previous findings^17,18,22, we show that knocking down alg-1 in adult worms reduces lifespan and impairs resistance to pro-oxidant agents. These phenotypes are accompanied by increases in sod-3 and gst-4 promoter activities in alg-1 deficient worms. Interestingly, the level of induction of these oxidative stress sensors in worms treated with alg-1 RNAi is like that obtained after exposure to paraquat, and the level of the sod-3 promoter activity in worms where alg-1 is knocked down is reduced in the presence of the antioxidant NAC, agreeing with a chronic state of oxidative stress in these worms.

One hypothesis to explain the overall dysfunction in redox homeostasis in adult worms deficient in alg-1 is the fact that DAF-16 activity is inhibited when ALG-1 function is lost¹⁷. DAF-16 orchestrates multiple stress response pathways in C. elegans, including oxidative stress response^50,51, and is involved in various longevity pathways such as those triggered by defects in insulin/IGF1 signaling or germline ablation^52–54. DAF-16 inhibition could render worms more prone to suffer from oxidative stress and thereby have a shorter lifespan. However, alg-1 deficiency further decreases the lifespan of daf-16 loss-of-function mutants¹⁷. In addition, most of the genes differentially expressed in alg-1(gk214) mutants are upregulated (consistent with a defect in miRNA biogenesis/function) and are not targets of DAF-16¹⁷, indicating that there are additional players downstream of ALG-1 that may participate in stress regulation and longevity.

While loss-of-function models of alg-1 can provide valuable insights into the fundamental role of ALG-1 in maintaining overall health, alg-1 deficiency is expected to disrupt multiple biological processes, and increased stress might reflect these widespread alterations, making it difficult to pinpoint how changes in ALG-1 physiologically control aging and stress response. Therefore, we searched conditions in which ALG-1 expression is induced and thus used gain-of-function models to investigate how ALG-1 upregulation affects longevity and stress resistance. We observed that ALG-1 is upregulated in various long-lived mutants [i.e., glp-1(e2141), clk-1(qm30), eat-2(ad1116), and raga-1(ok386)], but not in the insulin/IGF1 signaling deficient mutant age-1(hx546). Intermittent fasting, another life-extension intervention, also leads to alg-1 induction in C. elegans⁵⁵.

Guided by the modENCODE data, we performed RNAi screen on alg-1::gfp reporter strains to validate alg-1 regulators. We found that the transcription regulators GEI-2/MEP-1, NHR-77, and R02D3.7 negatively control ALG-1 levels in two distinct reporter strains. However, while nhr-28 or skn-1 RNAi was found to derepress alg-1 in the CT20 ALG-1 reporter strain (generated by transgene insertion), it did not affect ALG-1 levels in the PQ530 strain (generated by CRISPR engineering). Hence, RNAi targeting nhr-28 or skn-1 could be influencing ALG-1 levels in the CT20 strain via unspecific mechanisms (for instance, inhibition of transgene silencing⁵⁶).

Among the genes encoding these transcription regulators, only R02D3.7 is consistently downregulated in all long-lived mutants where alg-1 is upregulated, suggesting its importance as a key factor in controlling alg-1 expression in the context of longevity. Corresponding with its role in oxidative stress resistance, the knockdown of R02D3.7 enhances survival in sodium arsenite and paraquat stress assays. Notably, the impact of R02D3.7 on arsenite survival is entirely reliant on ALG-1, while its contribution to paraquat resistance appears to extend beyond ALG-1. Conversely, like the observed effects upon ALG-1 overexpression, RNAi targeting R02D3.7 fails to extend lifespan under normal conditions. R02D3.7 is a transcription factor carrying the well-conserved C2H2-type zinc finger motif. A study has recently described R02D3.7 as a negative regulator of cat-1 and cat-2 – genes involved in dopamine metabolism in C. elegans - rendering it the name RCAT-1 (regulator of cat genes)⁵⁷. Interestingly, R02D3.7 was identified as responsive to the pheromone ascaroside, which normally serves as a signal of starvation or overcrowding in C. elegans⁵⁷. Altogether, these results point to R02D3.7/RCAT-1 as a stress sensor controlling alg-1 transcription and stress response in C. elegans.

The alg-1 transcript can also be regulated in trans by miRNAs. One such miRNA is miR-71, which targets alg-1 and acts in a negative feedback loop to control miRNA biogenesis/function (this work and Inukai et al.²¹). miR-71 has been shown to promote lifespan and stress response in C. elegans (this work and de Lencastre et al.⁸), and longevity of glp-1 mutants depends on miR-71⁹. Although miR-71 is not increased when ALG-1 is overexpressed (i.e., CT20 worms), the levels of miR-71 are higher in glp-1 mutants. This indicates upregulation of ALG-1 in glp-1 mutants is not sufficient to increase miR-71, pointing to an additional mechanism to stabilize this miRNA in worms lacking the germline. Consistent with this hypothesis, there are twice as many miRNAs upregulated in glp-1 mutants than in ALG-1/OE worms. There are multiple steps in miRNA biogenesis that can be subjected to regulation for specific miRNAs to be stabilized. One of them is through the regulation of pri-miRNA transcription. Indeed, we identified the transcription factor GEI-2 as a positive regulator of the mir-71 promoter and found that gei-2 loss-of-function requires miR-71 to induce ALG-1, possibly by alleviating the suppressive effect miR-71 exerts over ALG-1. However, gei-2 is downregulated in glp-1 mutants, and gei-2 RNAi does not induce ALG-1 in these mutants. Hence, miR-71 levels are increased in glp-1 mutants despite the reduction of gei-2. These findings support an alternative mechanism stabilizing miR-71 in glp-1 mutants and reveal an intricate network controlling ALG-1 abundance at multiple levels. However, the level of induction of ALG-1 caused by the downregulation of R02D3.7 and potentially other mechanisms is strong enough to overcome the upregulation of miR-71 (and potentially other negative regulators of ALG-1) in glp-1 mutants. This mechanism allows the long-lived, stress-resistant glp-1 mutant to induce miRNA biogenesis/function by upregulating ALG-1 despite maintaining high levels of miR-71^9,13.

Considering that upregulation of miR-71 is sufficient to promote longevity⁹, the fact that miR-71 is not induced upon ALG-1 overexpression could also explain why ALG-1/OE worms are not long-lived under normal conditions (this work and Aalto et al.¹⁷). On the other hand, we observed that ALG-1 overexpression mimics the oxidative stress resistance phenotype of the germline-deficient mutant glp-1, one of the long-lived mutants that displays the highest level of ALG-1. Elevated levels of ALG-1 also delay larval development and reduce brood size. Similarly, worms with loss-of-function mutation in alg-1 (allele gk214) exhibit various developmental impairments, including heterochronic defects and reduced progeny^16,58, while being short-lived^17,18. These results underline the importance of ALG-1 and miRNAs in development and reproduction, and suggest that miRNA regulation may play a crucial role controlling the balance between reproduction and somatic maintenance⁵⁹.

ALG-1 overexpression only increases lifespan when worms are cultured in bacteria that do not produce NO. Considering that C. elegans lacks nitric oxide synthase, the only source of NO worms are exposed to derive from the bacteria³². NO inhibits ALG-1 post-translationally via S-nitrosylation³⁰. Hence, the absence of NO could further stimulate ALG-1 function. NO is also a free radical known to participate in redox mechanisms and reacts with superoxide^35,60. Hence, in an NO-free environment, worms are expected to suffer from redox alterations, which include increases in superoxide levels and overreliance on superoxide dismutases to maintain redox balance, a condition that could sensitize worms to respond to ALG-1 overexpression.

In agreement, ALG-1 overexpression renders C. elegans more resistant to stress and this protection appears to be specific to oxidative stress, since ALG-1/OE does not protect worms from temperature stress and sensitizes them to reductive stress by DTT, further indicating that ALG-1 controls redox balance by pushing it towards a more reductive state. Our observations agree with a previous study by Finger et al. who show that ALG-1 is required for proper oxidative stress resistance in C. elegans¹⁸. On the other hand, in their model of alg-1 loss-of-function, they observed decreased heat stress resistance and impaired proteostasis. Together, these results suggest that while alg-1 deficiency reduces lifespan and increases vulnerability to multiple stressors, ALG-1 overexpression selectively improves survival under oxidative stress. Moreover, the complexity of the response and the intricate regulatory mechanism that ALG-1 is subjected to indicate that ALG-1 can be dynamically altered to confer oxidative stress protection, but should also be tightly regulated not to compromise other stress responses.

A plausible mechanism to explain how ALG-1 induction might confer protection against oxidative stress involves the upregulation of mitochondrial superoxide dismutase SOD-3. ALG-1 overexpression, like alg-1 knockdown, induces the sod-3 promoter. However, adding the antioxidant NAC to ALG-1/OE worms does not inhibit sod-3 promoter activity, as it does in worms exposed to alg-1 RNAi. This supports the notion that higher levels of ALG-1 preventively enhance sod-3 promoter activity independently of endogenous pro-oxidant levels, aiding worms to endure oxidative stress. Consistent with these observations, glp-1 mutants exhibit higher SOD-3 levels and have improved oxidative stress response (this study and^11,13). Additionally, we demonstrated that the increased oxidative stress resistance of glp-1 mutants is dependent on alg-1. Furthermore, while DAF-16 and SKN-1 contribute to the prolonged lifespan and stress resistance of glp-1 mutants^{13,39,41,53,61}, the protective effects facilitated by ALG-1 overexpression also occur in conditions where daf-16 and skn-1 are silenced^{11,13,39,41,53}. Together, these findings suggest that the upregulation of ALG-1 operates in tandem with DAF-16 and SKN-1, collectively enhancing stress resistance in germline-deficient mutants, in part manifested by upregulation of sod-3.

Contrasting previous data from the literature showing that mir-71 loss-of-function mutants are more sensitive to oxidative stress⁸, we did not see differences between the mir-71(n4115) null mutant and control worms under paraquat or sodium arsenite, although in our experiments the worms carried additional transgenes. Nevertheless, loss of mir-71 blunted the oxidative stress protection promoted by ALG-1/OE. These results show that normal levels of miR-71 are required for stress resistance of worms overexpressing ALG-1. However, our model also contemplates the possibility that miRNAs other than miR-71 are playing a dynamic role in controlling oxidative stress response after upregulation of ALG-1. To identify these players, we measured miRNAs commonly upregulated in glp-1 mutants and ALG-1/OE worms. Besides playing a fundamental role in the function of miRNAs, ALG-1 also participates in miRNA biogenesis by stabilizing the guide strand of miRNAs. In agreement, ALG-1 deficiency decreases global miRNA levels^15,16 and most of the miRNAs that fell within our cut-off (log₂ fold change > 1 or < −1) were upregulated in ALG-1/OE worms and glp-1 mutants. Of 11 miRNAs commonly upregulated in the two conditions, we showed that disruption of the mir-87, mir-230, and mir-235 genes sensitized worms to oxidative stress. Interestingly, these miRNAs are also upregulated in the dietary-restricted, long-lived mutant eat-2⁶². Moreover, miR-230-3p expression is increased in response to heat stress⁶³, while its expression decreases in aged worms²¹. miR-235-3p is also downregulated in aged worms, and mediates longevity induced by dietary restriction in C. elegans⁶⁴. mir-235 also has a protective effect on the response to exposure to graphene oxide⁶⁵, a toxic agent. These findings unveiled miRNAs induced by ALG-1 overexpression as relevant players in oxidative stress response.

Among the putative targets of these miRNAs, we found genes that are predicted to have their molecular function associated with PDI activity. PDIs are multifunctional enzymes with oxidoreductase, isomerase, and chaperone activities. PDI promotes the formation of disulfide bonds in newly synthesized ER proteins, primarily those destined to secretion or to the cell surface⁶⁶. The thiol oxidase function of PDI is intricately linked to its reoxidation by ER oxidoreductin-1 (Ero1). This process involves the generation of reduced Ero1, which subsequently needs to be regenerated to its oxidized form. This regeneration occurs through electron transfer from reduced Ero1 to O₂, leading to the generation of hydrogen peroxide⁶⁶.

The ER lumen is known for its relatively oxidizing environment, characterized by high concentrations of hydrogen peroxide⁶⁷. Concurrently, Ero1-dependent catalysis relies on the reduction of its non-catalytic regulatory disulfides, a process involving PDI or glutathione⁶⁸. Thus, the loss of PDI may limit Ero1 activity, providing some level of protection against oxidative stress. However, this protective effect may come at the cost of impaired protein folding capacity, while simultaneously rendering cells more susceptible to reductive stress. Additional mechanisms associated with the effects of PDI depletion may include the loss of oxidized glutathione in the ER⁶⁸ and a diminished supportive interaction between PDI and oxidant-generating Nox NADPH oxidases⁶⁶. These possible mechanisms remain to be investigated. On the other hand, general induction of miRNAs by upregulation of ALG-1 is anticipated to have a broad inhibitory effect on protein synthesis. Hence, ALG-1 upregulation and consequent downregulation of the PDI pathway may alter ER redox regulation and protein folding capacity through multiple mechanisms.

These observations concur with the fact that worms overexpressing ALG-1 are more sensitive to ER stress induced by the reducing agent DTT, while they cope better with exogenous exposure to pro-oxidant agents. In C. elegans, PDI-1, PDI-2, PDI-3, and PDI-6 are the best-characterized PDI proteins with homologies to human PDIs⁶⁹. We found that miR-230-3p can directly target pdi-2. C. elegans mutants with loss-of-function of pdi-2 exhibit severe morphological defects, uncoordinated movement, and adult sterility⁷⁰.

Here we used heterozygous mutants resulting in partial inhibition of pdi-2 and we observed that limiting the enzyme improves oxidative stress resistance. Knockdown of pdi-2 using RNAi results in similar protection from paraquat stress. Curiously though, pdi-2 RNAi not only sensitizes worms to sodium arsenite, but also results in decreased lifespan under normal, unstressed conditions. These findings underscore the critical importance of fine-tuning the regulation of PDI-2. Taking into consideration the important role of PDI in maintaining redox balance in the ER while conferring proper protein homeostasis, it is expected that drastic changes in PDI-2 levels will lead to deleterious effects. Hence, whether pdi-2 inhibition proves beneficial or detrimental may be a matter of the magnitude and the duration of the repression, as well as the nature of the stress.

Previous studies have indicated that neurons in C. elegans exhibit resistance to RNAi^71,72, whereas the pdi-2 mutation is anticipated to impact all cells. Consequently, the varying outcomes observed with different loss-of-function models may also signify the influence of distinct tissues on the phenotypes. Given the tissue specificity of many miRNAs⁷³ and their established role in fine-tuning gene networks⁵, we posit that miRNAs serve as cellular guardians of the PDI pathway, preventing unbalanced changes that could lead to cellular dysfunction during stressful conditions, consequently influencing organismal stress resistance.

In conclusion, in the present work we described the mechanism through which the miRNA processing machinery is dynamically regulated to orchestrate organismal oxidative stress resistance under several conditions that lead to longevity, particularly in germline-deficient animals. Under a pro-oxidant environment (common in disease conditions), increasing a key enzyme that represents a limiting factor for miRNA function and biogenesis promotes survival of the organism. Importantly, increasing the efficiency of the miRNA machinery is not always beneficial, as it can also sensitize the organism to other kinds of stressors, decrease reproductive output, and delay development. Hence, it is not surprising that the physiological regulation of ALG-1 is tightly controlled by an intricate mechanism. Although some of the players participating in this mechanism as described here in C. elegans are not fully conserved, the tight regulation of components of the miRNA processing pathway and their role in stress response and aging have been clearly demonstrated in mammals^47,74–76. In humans, germline mutations in argonautes (AGO1 and AGO2) have been associated with defects in neurodevelopment^77,78, while somatic mutations in AGO2 appear to be common in gastric and colorectal cancers with high microsatellite instability⁷⁹. Future studies could reveal whether targeting these specific argonautes may serve to treat diseases associated with oxidative stress and improve human health.

Methods

Strains and maintenance of C. elegans

C. elegans were obtained from the Caenorhabditis Genetics Center (CGC). Worms were maintained in Petri dishes containing semi-solid Nematode Growth Media (NGM) supplemented with 1 mM CaCl₂, 1 mM MgSO₄, 25 mM KPO₄ and 5 µg/mL cholesterol, as described previously⁸⁰. The NGM medium was supplemented with 100 μg/mL of streptomycin (Sigma-Aldrich, S6501-25G) for the maintenance plates seeded with OP50-1 (a streptomycin-resistant strain of OP50 E. coli), to avoid contamination. Bacteria were grown for 16 hours, during which they reached an optical density of approximately 1. Then, the culture was concentrated 10 times and inoculated onto plates containing NGM, forming a lawn above which the worms were cultivated. All C. elegans strains used are summarized in Supplementary Table 1. We used hermaphrodites in all experiments and males only for mating.

RNAi

For RNAi experiments, NGM plates were supplemented with 1 mM CaCl₂, 1 mM MgSO₄, 25 mM KPO₄, 8 µg/mL cholesterol, 12.5 µg/mL tetracycline (Sigma-Aldrich, T7660), 100 µg/mL ampicillin (Sigma-Aldrich, A9518), and 1 mM Isopropyl-β-D-thiogalactopyranoside (IPTG) (Fisher Scientific, BP1755-1) to induce double-stranded RNA expression. C. elegans were fed with HT115 E. coli bacteria expressing the RNAi clones, which were obtained from the C. elegans ORFeome Library (Vidal RNAi library available through Horizon Discovery), kindly provided by Dr. Adam Antebi and Dr. Julio Ferreira. For control (ctrl) RNAi, HT115 expressing the L4440 (empty vector) clone was used.

Lifespans assays

Approximately 120 synchronized day 0 (young adults) worms were transferred to lifespan plates containing E. coli OP50-1 (streptomycin-resistant strain) or E. coli HT115 (for RNAi experiments) bacteria and supplemented with 50 µg/mL 5-Fluoro-2’-deoxyuridine (FudR) (Thermo Scientific Chemicals, 227605000). Lifespans were performed at 20 °C under normal conditions. For lifespans under NO-free conditions, B. subtilis strain 1A1 (strain 168) and the isogenic B. subtilis ΔNOS, obtained from the Bacillus Genetic Stock Center (BGSC), were used. For lifespans under heat stress, a temperature of 30 °C was used. For oxidative stress induced by methyl viologen dichloride hydrate (Paraquat) (Sigma-Aldrich, 856177), worms were transferred at L4 stage to lifespan plates supplemented with either 4 mM (for OP50-1 bacteria) or 8 mM of Paraquat (for HT115 bacteria). For reductive ER stress induced by DTT (dithiothreitol) (Thermo Fisher Scientific, D0632), the C. elegans strains were transferred at day 0 young adults to lifespan plates supplemented with 5 mM DTT. For all lifespans, dead worms were scored every 1 to 2 days from day 1, and animals that died by bagging, bursting, or crawling off the plates were censored.

Oxidative stress induced by sodium arsenite

Using 96-well plates, day 3 adult worms were transferred to wells containing 100 µL of sodium arsenite (Sigma-Aldrich, S7400) solution in concentrations ranging from 10 to 15 mM, diluted in M9 buffer (22 mM Na₂HPO₄, 22 mM KH₂PO₄, 85 mM NaCl, 1 mM MgSO₄). After 8 h, dead worms were scored by touching their tail three times with a platinum wire. When touch response was absent, worms were considered dead. At least 6 wells containing 10 worms were used for each strain and each concentration. The experiments were repeated at least 2 times.

Mobility analysis

Mobility was measured on days 0, 3, 6, and 9 of adulthood. Ten worms from lifespan plates were placed, individually, in a well of a 96-well plate containing 100 µL of M9 buffer and left at 20 °C for 10 min to acclimatize. The number of body bends per worm was measured for 30 s using a light stereoscope, and the values were multiplied by 2 to obtain the rate per minute. The measurements were repeated twice per worm and data represents the average.

Pharyngeal pumping

Pharyngeal pumping analysis was done on days 0, 3, 6, and 9 of adulthood. Ten worms had their pharynx movements on lifespan plates observed using a light stereoscope. The number of pharynx movements per worm was measured for 30 s, and the values were multiplied by 2 to obtain the rate per minute. The measurements were repeated twice per worm and data represents the average.

Duration of development

Individual adult worms were allowed to lay eggs for one hour on OP50-1 plates. After 60 hours of progeny development, the plates were monitored every hour using a light stereoscope to score for adults, identified by the presence of eggs in the uterus. This monitoring continued until the last worm reached the adult stage.

Brood size assay

Approximately 200 eggs laid by adult worms were transferred to OP50-1 plates and maintained until day 0 (young adults). Each adult worm was then individually transferred to new plates and maintained for 24 hours. After 24 hours, the worms were transferred to fresh wells for another 24-hour incubation, while the eggs/larvae from the previous well were counted. This procedure was repeated until day 5 of adulthood.

ModENCODE analysis

To look for candidates for alg-1 transcriptional regulators, version 33 of the modENCODE ChIP-Sequencing consortium²⁴ was used. The candidates were picked by selecting genes that had a significant peak in the region of up to 2000 base pairs upstream of alg-1 initiation codon (X chromosome: 13947420..13949420).

GFP reporter analyses

For measurements of the alg-1p::alg-1::gfp reporter (ap423 allele obtained from the PQ530 strain) in the long-lived mutants, the strains were maintained on OP50-1, and had their fluorescence measured on day 1 of adulthood. Ten to twenty worms were immobilized using 0.1% sodium azide (Sigma-Aldrich, 71290) on M9 solution and placed on glass slides. The images were acquired using the ZEISS Apotome 3 (Zeiss microscopy). For experiments using the other reporters, the strains were transferred to plates containing 50 µg/mL FudR (Thermo Scientific Chemicals, 227605000) on day 0 of adulthood. For sod-3 and gst-4 analyses, plates were also supplemented with 4 mM Paraquat (Sigma-Aldrich, 856177), 10 mM N-acetylcysteine (NAC) (Sigma-Aldrich, A7250) or vehicle (M9) solution. On day 3 of adulthood, ten adult worms were transferred to transparent 96-well plates containing 100 µL of 0.1% sodium azide (Sigma-Aldrich, 71290) in M9 buffer, for immobilization, and had their images acquired using Cytation™ 5 Cell Imaging Multi-Mode Reader (BioTek Instruments). For all measurements using RNAi, worms were grown on ctrl RNAi (empty vector) plates until day 0 and then transferred to the experimental RNAi until the day fluorescence was measured. The software ImageJ Fiji (National Institute of Health) was used for image analysis. The mean fluorescence intensity of each worm was calculated, and the normalization was performed by subtracting the mean intensity values of worms without fluorescence (WT) and dividing these values by the mean intensity values of the control group.

Real-time qPCR

RNA from 300 day-1 adult worms was extracted using TRIzol Reagent (Thermo Fisher Scientific, 15596018). Reverse transcription was performed using 200 ng of total RNA and High-Capacity cDNA Reverse Transcription kit (Thermo Fisher Scientific, 4368814) according to the manufacturer’s protocol. Real-time PCR was conducted using SYBR Green Master Mix (Thermo Fisher Scientific, 4309155) and primers at the final concentration of 0.5 μM. Fluorescence was detected using the CFX384 Detection System (Bio-Rad Laboratories). Real-Time PCR System following the protocol: 95 °C−5 min and 40 cycles of 95 °C−15 s, 60 °C−20 s, and 72 °C−30 s. Expression levels were normalized using the reference gene Y45F10D.4. Primers used: alg-1 forward - CGCGCTCGTTAATCATCTTGT, alg-1 reverse - GGATGAACCTGCACAGCTC, Y45F10.4 forward - CGAGAACCCGCGAAATGTCGGA, Y45F10.4 reverse - CGGTTGCCAGGGAAGATGAGGC.

Small RNA sequencing

Total RNA was extracted from pools of 500–800 C. elegans at day 0 using TRIzol reagent and following the manufacturer’s instructions (Thermo Fisher Scientific, 15596018). Samples of 6 µg of total RNA were sent for small RNA sequencing at the Genomics Center of ESALQ-USP using the HiSeq2500 platform (Illumina). After preprocessing the data with the Fastx-ToolKit software to remove adapters and select reads with a minimum length of 18 base pairs (bp), the analysis was conducted using the Bowtie2 software with the ce10 reference genome provided by UCSC. The data was normalized by the total number of reads generated per sample. miRNAs with log₂ fold change > 1 or < −1 when comparing to their control groups [N2 for glp-1(e2144) and ctrl for ALG-1/OE] were considered differentially expressed and were plotted in a heatmap generated using GraphPad Prism (version 8.0). Venn diagrams were created using the following website: http://bioinformatics.psb.ugent.be/webtools/Venn/. The complete raw data can be accessed through the Gene Expression Omnibus (GEO) by the accession number GSE260938.

RNAseq data analysis

RNAseq data (GSE111338) was assessed at GEO and used to retrieve gene expression data of glp-1(e2141) vs. WT worms at day 1. For eat-2(ad1116), raga-1(ok386), clk-1(qm30), and age-1(hx546) mutants at day 1, we used the RNAseq data from Dutta et al.²³, available upon request from the Mair lab. Statistical analysis was performed using EdgeR package, on RStudio (version 1.3.1). The data were normalized with “calcnormFactors()” using the “glmQLFTest()” method. Data were considered statistically different when P value and false discovery rate (FDR) were less than 0.05.

Gene ontology of miRNA targets

The TargetScanWorm Release 6.2⁴⁴ was used to assess predicted miRNA targets. Predicted targets with aggregate Pct > 0.19 were selected and intersected with genes upregulated on a microarray of alg-1(gk214) worms⁴⁵ (GSE19138) curated by WormExp v2.0⁸¹. The list of intersected genes had their gene ontology analyzed on WormEnrichr⁴⁶, using the gene set library GO molecular function AutoRIF Predicted z-score.

pdi-2 3’UTR cloning

To clone the putative binding site of miR-230-3p located at the pdi-2 3’UTR into the 3’UTR of a luciferase reporter vector, oligonucleotides (pdi-2 sense CTAGTTAGCGGCCGCTAGTATCATCTCATCTTTACTAATAAA; pdi-2 antisense AGCTTTccggtcTAAAGATGAccTGATACTAGCGGCCGCTAA; mutated pdi-2 sense CTAGTTAGCGGCCGCTAGTATCAggTCATCTTTAgaccggAA; mutated pdi-2 antisense AGCTTTccggtcTAAAGATGAccTGATACTAGCGGCCGCTAA) were synthesized, diluted to a concentration of 1 µg/µL and annealed in annealing buffer (10 mM Tris, pH 7.5 − 8.0; 50 mM NaCl; 1 mM EDTA). The solution was heated at 95 °C for 2 min, allowed to cool to room temperature and kept in this condition for 45 min. 1 µg of pMIR-REPORT^TM vector (Thermo Fisher Scientific, AM5795) was digested with 1 µL (10 units) of restriction enzymes SpeI (New England Biolabs, NEB #R3133) and HindIII (New England Biolabs, NEB #R3104), in the presence of Cutsmart buffer (New England Biolabs, NEB #B6004), to a final volume of 50 µL. The annealed oligos were diluted to 4 ng/µL and ligated to 50 ng of pMIR-REPORT, in the presence of T4 DNA ligase (New England Biolabs, M0202S) and 1x ligase buffer (New England Biolabs, B0535S) in a final volume of 20 µL. 2 µl of the ligation was transformed into competent DH5α bacteria according to the Addgene protocol (https://www.addgene.org/protocols/bacterial-transformation) and then 100 µL of the transformation were plated on LB-agar plates containing 100 mg/mL of ampicillin (Sigma-Aldrich, A9518-25g). Clones were selected and plasmids were isolated using the QIAprep Spin miniprep kit (Qiagen, 27104).

miR-230-3p target assay

HEK293T cells were seeded into 96-well plates and, after 24 hours, they were transfected with plasmids carrying the luciferase gene under the control of the native or mutated pdi-2 3’UTR sequences (1 µg/mL) in the presence of the C. elegans miR-230-3p (Thermo Scientific, 4464066) or miR-85-3p (negative control) (Thermo Scientific, 4464066) mimics at the concentration of 17.5 nM. The vector pRL-SV40 (which expresses Renilla luciferase) was co-transfected for normalization. Plasmids were transfected using the Effectene Transfection Reagent kit (Qiagen, 301425) and miRNA mimics using the HiPerFect Transfection Reagent kit (Qiagen, 301704). After 24 hours of transfection medium was exchanged, and 24 hours later the cells were washed with PBS and luminescence of Firefly Luciferase and Renilla Luciferase was measured using the Dual-Glo® Luciferase Assay kit (Promega, E2920).

Statistics

Lifespan assays were compared using the log-rank test. Two-tailed Student’s t-test was used to compare two means, and one-way ANOVA was used to compare more than two means. In experiments with two independent variables, means were compared using two-way ANOVA. We assumed normal distribution for statistical comparisons. GraphPad Prism (version 8.0) was used to plot data and to calculate statistics. P < 0.05 was considered statistically significant.

Reporting summary

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

Supplementary information

Supplementary Information^{(10MB, pdf)}

Peer Review File^{(1.9MB, pdf)}

41467_2024_47306_MOESM3_ESM.pdf^{(109.4KB, pdf)}

Description of Additional Supplementary Files

Supplementary Data 1^{(16.5KB, xlsx)}

Supplementary Data 2^{(16.5KB, xlsx)}

Supplementary Data 3^{(26.3KB, xlsx)}

Supplementary Data 4^{(126.5KB, xlsx)}

Reporting Summary^{(2.1MB, pdf)}

Source data

Source Data^{(1.3MB, xlsx)}

Acknowledgements

We thank Elzira E. Saviani and Anne Lanjuin for technical support, and the C. elegans Genetics Center (University of Minnesota) – funded by the NIH Office of Research Infrastructure Programs (P40 OD010440) – for providing C. elegans strains. We also thank the Genomics Center of ESALQ-USP for the small RNA sequencing, and Adam Antebi (Max Planck Institute for Biology of Ageing) and Julio Ferreira (University of São Paulo) for RNAi clones. We thank Franscisco Laurindo (University of São Paulo) for reagents and discussion. This work was funded by the Conselho Nacional de Desenvolvimento Científico e Tecnológico (CNPq) – grant number 310287/2018-9 (M.A.M.), Coordenação de Aperfeiçoamento de Pessoal de Nível Superior – Brasil (CAPES) – Finance Code 001, 88887.340135/2019-00 (C.A.V.J), 88887.489628/2020-00 (G.T.S), 88881.143924/2017-01 (M.A.M.), Fundação de Amparo à Pesquisa do Estado de São Paulo (FAPESP) – grant numbers: 2019/01587-1 (C.A.V.J), 2016/15958-3 (R.P.M.), 2017/04377-2 (S.P.), 2023/08316-9 (E.A.S.), 2022/05851-8 (E.A.S.), 2014/10814-8 (E.A.S.), 2017/01339-2 (H.C.), 2018/11792-9 (D.L.B), 2019/04726-2 (T.L.K), 2018/21635-8 (G.P.R.), 2017/23920-9 (R.G.L.), 2014/50897-0 (K.B.M.), 2021/08354-2 (M.A.M.), 2019/25958-9 (M.A.M.), 2017/01184-9 (M.A.M.), and National Institutes on Aging - R01AG044346, R01AG059595 (W.B.M).

Author contributions

C.A.V.J.: Conceptualization, Formal analysis, Investigation, Writing – Original Draft, Visualization, Project administration; R.P.M.: Conceptualization, Formal analysis, Investigation, Project administration, Review & Editing; S.P.: Investigation, Validation, Review & Editing; E.A.S.: Investigation, Validation, Review & Editing; H.C.: Conceptualization, Investigation, Review & Editing; D.L.B.: Investigation, Validation; G.T.S.: Investigation, Validation, Review & Editing; T.L.K.: Investigation, Validation; G.P.R.: Investigation, Validation; R.G.L.: Investigation, Validation; K.B.M.: Resources provision, Funding acquisition, Review & Editing; W.B.M.: Conceptualization, Review & Editing, Resources provision; M.A.M.: Conceptualization, Writing – Review & Editing, Project administration, Funding acquisition, Resources provision.

Peer review

Peer review information

Nature Communications thanks the anonymous reviewer(s) for their contribution to the peer review of this work. A peer review file is available.

Data availability

All data generated or analyzed during this study are provided in the Supplementary Information and Source Data files and are available in public repositories or upon request from their original sources. The small RNA sequencing data generated in this study (Fig. 4a–e) have been deposited in the GEO database under accession code GSE260938. The processed data is also available in the Supplementary Data 3. The RNA sequencing data re-used in this study (Fig. 1a, g and Supplementary Fig. 2a) are available in the GEO database under accession code GSE111338 or were shared by and is available upon request from the Mair lab²³. The processed data used in the study are also available in the Supplementary Data 1. The microarray data re-used in this study (Fig. 5a and Supplementary Fig. 9) are available in the GEO database under accession code GSE19138. The processed data used in this study is also available in the Supplementary Data 4. Source data are provided with this paper.

Competing interests

The authors declare no competing interests.

Footnotes

Publisher’s note Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

These authors contributed equally: Carlos A. Vergani-Junior, Raíssa De P. Moro.

Supplementary information

The online version contains supplementary material available at 10.1038/s41467-024-47306-4.

References

1.López-Otín C, Blasco MA, Partridge L, Serrano M, Kroemer G. Hallmarks of aging: An expanding universe. Cell. 2023;186:243–278. doi: 10.1016/j.cell.2022.11.001. [DOI] [PubMed] [Google Scholar]
2.Pomatto LCD, Davies KJA. The role of declining adaptive homeostasis in ageing. J. Physiol. 2017;595:7275–7309. doi: 10.1113/JP275072. [DOI] [PMC free article] [PubMed] [Google Scholar]
3.Blackwell TK, Steinbaugh MJ, Hourihan JM, Ewald CY, Isik M. SKN-1/Nrf, stress responses, and aging in Caenorhabditis elegans. Free Radic. Biol. Med. 2015;88:290–301. doi: 10.1016/j.freeradbiomed.2015.06.008. [DOI] [PMC free article] [PubMed] [Google Scholar]
4.Kenyon CJ. The genetics of ageing. Nature. 2010;464:504–512. doi: 10.1038/nature08980. [DOI] [PubMed] [Google Scholar]
5.Bartel DP. Metazoan MicroRNAs. Cell. 2018;173:20–51. doi: 10.1016/j.cell.2018.03.006. [DOI] [PMC free article] [PubMed] [Google Scholar]
6.Boehm M, Slack F. A developmental timing MicroRNA and its target regulate life span in C. elegans. Science. 2005;310:1954–1957. doi: 10.1126/science.1115596. [DOI] [PubMed] [Google Scholar]
7.Elder CR, Pasquinelli AE. New roles for MicroRNAs in old worms. Front. Aging. 2022;3:871226. doi: 10.3389/fragi.2022.871226. [DOI] [PMC free article] [PubMed] [Google Scholar]
8.de Lencastre A, et al. MicroRNAs both promote and antagonize longevity in C. elegans. Curr. Biol. 2010;20:2159–2168. doi: 10.1016/j.cub.2010.11.015. [DOI] [PMC free article] [PubMed] [Google Scholar]
9.Boulias K, Horvitz HR. The C. elegans MicroRNA mir-71 Acts in Neurons to Promote Germline-Mediated Longevity through Regulation of DAF-16/FOXO. Cell Metab. 2012;15:439–450. doi: 10.1016/j.cmet.2012.02.014. [DOI] [PMC free article] [PubMed] [Google Scholar]
10.Finger F, et al. Olfaction regulates organismal proteostasis and longevity via microRNA-dependent signalling. Nat .Metab. 2019;1:350–359. doi: 10.1038/s42255-019-0033-z. [DOI] [PMC free article] [PubMed] [Google Scholar]
11.Wei Y, Kenyon C. Roles for ROS and hydrogen sulfide in the longevity response to germline loss in Caenorhabditis elegans. Proc. Natl Acad. Sci. 2016;113:E2832–E2841. doi: 10.1073/pnas.1524727113. [DOI] [PMC free article] [PubMed] [Google Scholar]
12.Arantes-Oliveira N, Apfeld J, Dillin A, Kenyon C. Regulation of life-span by germ-line stem cells in Caenorhabditis elegans. Science. 2002;295:502–505. doi: 10.1126/science.1065768. [DOI] [PubMed] [Google Scholar]
13.Steinbaugh MJ, et al. Lipid-mediated regulation of SKN-1/Nrf in response to germ cell absence. Elife. 2015;4:e07836. doi: 10.7554/eLife.07836. [DOI] [PMC free article] [PubMed] [Google Scholar]
14.Youngman EM, Claycomb JM. From early lessons to new frontiers: the worm as a treasure trove of small RNA biology. Front. Genet. 2014;5:416. doi: 10.3389/fgene.2014.00416. [DOI] [PMC free article] [PubMed] [Google Scholar]
15.Zinovyeva AY, Bouasker S, Simard MJ, Hammell CM, Ambros V. Mutations in conserved residues of the C. elegans microRNA Argonaute ALG-1 identify separable functions in ALG-1 miRISC loading and target repression. PLoS Genet. 2014;10:e1004286. doi: 10.1371/journal.pgen.1004286. [DOI] [PMC free article] [PubMed] [Google Scholar]
16.Grishok A, et al. Genes and mechanisms related to RNA interference regulate expression of the small temporal RNAs that Control C. elegans developmental timing. Cell. 2001;106:23–34. doi: 10.1016/S0092-8674(01)00431-7. [DOI] [PubMed] [Google Scholar]
17.Aalto AP, et al. Opposing roles of microRNA Argonautes during Caenorhabditis elegans aging. PLoS Genet. 2018;14:e1007379. doi: 10.1371/journal.pgen.1007379. [DOI] [PMC free article] [PubMed] [Google Scholar]
18.Finger, F., Ottens, F. & Hoppe, T. The Argonaute Proteins ALG-1 and ALG-2 Are Linked to stress resistance and proteostasis. MicroPubl. Biol. v.2021, 10.17912/micropub.biology.000457 (2021). [DOI] [PMC free article] [PubMed]
19.Pagliuso DC, Bodas DM, Pasquinelli AE. Recovery from heat shock requires the microRNA pathway in Caenorhabditis elegans. PLoS Genet. 2021;17:e1009734. doi: 10.1371/journal.pgen.1009734. [DOI] [PMC free article] [PubMed] [Google Scholar]
20.Bukhari SIA, et al. The microRNA pathway controls germ cell proliferation and differentiation in C. elegans. Cell Res. 2012;22:1034–1045. doi: 10.1038/cr.2012.31. [DOI] [PMC free article] [PubMed] [Google Scholar]
21.Inukai S, Pincus Z, De Lencastre A, Slack FJ. A microRNA feedback loop regulates global microRNA abundance during aging. RNA. 2018;24:159–172. doi: 10.1261/rna.062190.117. [DOI] [PMC free article] [PubMed] [Google Scholar]
22.Kato M, Chen X, Inukai S, Zhao H, Slack FJ. Age-associated changes in expression of small, noncoding RNAs, including microRNAs, in C. elegans. RNA. 2011;17:1804–1820. doi: 10.1261/rna.2714411. [DOI] [PMC free article] [PubMed] [Google Scholar]
23.Dutta, S. et al. Efficacy of longevity interventions in C. elegans is determined by early life activity of RNA splicing factors. bioRxiv 2021.11.01.466772 10.1101/2021.11.01.466772 (2021).
24.Gerstein MB, et al. Integrative Analysis of the Caenorhabditis elegans Genome by the modENCODE Project. Science. 2010;330:1775–1787. doi: 10.1126/science.1196914. [DOI] [PMC free article] [PubMed] [Google Scholar]
25.Chan S-P, Slack FJ. Ribosomal protein RPS-14 modulates let-7 microRNA function in Caenorhabditis elegans. Dev. Biol. 2009;334:152–160. doi: 10.1016/j.ydbio.2009.07.011. [DOI] [PMC free article] [PubMed] [Google Scholar]
26.Lagido C, Pettitt J, Flett A, Glover LA. Bridging the phenotypic gap: real-time assessment of mitochondrial function and metabolism of the nematode Caenorhabditis elegans. BMC Physiol. 2008;8:7. doi: 10.1186/1472-6793-8-7. [DOI] [PMC free article] [PubMed] [Google Scholar]
27.Pasquinelli AE, Ruvkun G. Control of Developmental Timing by MicroRNAs and Their Targets. Annu. Rev. Cell Dev. Biol. 2002;18:495–513. doi: 10.1146/annurev.cellbio.18.012502.105832. [DOI] [PubMed] [Google Scholar]
28.Lagos-Quintana M, Rauhut R, Lendeckel W, Tuschl T. Identification of novel genes coding for small expressed RNAs. Science. 2001;294:853–858. doi: 10.1126/science.1064921. [DOI] [PubMed] [Google Scholar]
29.Lau NC, Lim LP, Weinstein EG, Bartel DP. An abundant class of tiny RNAs with probable regulatory roles in Caenorhabditis elegans. Science. 2001;294:858–862. doi: 10.1126/science.1065062. [DOI] [PubMed] [Google Scholar]
30.Seth P, et al. Regulation of MicroRNA machinery and development by interspecies S-Nitrosylation. Cell. 2019;176:1014–1025.e12. doi: 10.1016/j.cell.2019.01.037. [DOI] [PMC free article] [PubMed] [Google Scholar]
31.Bito T, et al. Vitamin B12 deficiency results in severe oxidative stress, leading to memory retention impairment in Caenorhabditis elegans. Redox Biol. 2017;11:21–29. doi: 10.1016/j.redox.2016.10.013. [DOI] [PMC free article] [PubMed] [Google Scholar]
32.Gusarov I, et al. Bacterial nitric oxide extends the lifespan of C. elegans. Cell. 2013;152:818–830. doi: 10.1016/j.cell.2012.12.043. [DOI] [PubMed] [Google Scholar]
33.Hao Y, et al. Thioredoxin shapes the C. elegans sensory response to Pseudomonas produced nitric oxide. Elife. 2018;7:e36833. doi: 10.7554/eLife.36833. [DOI] [PMC free article] [PubMed] [Google Scholar]
34.Piacenza L, Zeida A, Trujillo M, Radi R. The superoxide radical switch in the biology of nitric oxide and peroxynitrite. Physiol. Rev. 2022;102:1881–1906. doi: 10.1152/physrev.00005.2022. [DOI] [PubMed] [Google Scholar]
35.Radi R. Oxygen radicals, nitric oxide, and peroxynitrite: Redox pathways in molecular medicine. Proc. Natl Acad. Sci. 2018;115:5839–5848. doi: 10.1073/pnas.1804932115. [DOI] [PMC free article] [PubMed] [Google Scholar]
36.Bus JS, Gibson JE. Paraquat: model for oxidant-initiated toxicity. Environ. Health Perspect. 1984;55:37–46. doi: 10.1289/ehp.845537. [DOI] [PMC free article] [PubMed] [Google Scholar]
37.Bagley AC, Krall J, Lynch RE. Superoxide mediates the toxicity of paraquat for Chinese hamster ovary cells. Proc. Natl Acad. Sci. 1986;83:3189–3193. doi: 10.1073/pnas.83.10.3189. [DOI] [PMC free article] [PubMed] [Google Scholar]
38.Guidarelli A, Fiorani M, Cerioni L, Cantoni O. The compartmentalised nature of the mechanisms governing superoxide formation and scavenging in cells exposed to arsenite. Toxicol. Appl. Pharmacol. 2019;384:114766. doi: 10.1016/j.taap.2019.114766. [DOI] [PubMed] [Google Scholar]
39.An JH, Blackwell TK. SKN-1 links C. elegans mesendodermal specification to a conserved oxidative stress response. Genes Dev. 2003;17:1882–1893. doi: 10.1101/gad.1107803. [DOI] [PMC free article] [PubMed] [Google Scholar]
40.Yamawaki TM, Arantes-Oliveira N, Berman JR, Zhang P, Kenyon C. Distinct activities of the germline and somatic reproductive tissues in the regulation of Caenorhabditis elegans’ longevity. Genetics. 2008;178:513–526. doi: 10.1534/genetics.107.083253. [DOI] [PMC free article] [PubMed] [Google Scholar]
41.Lin K, Hsin H, Libina N, Kenyon C. Regulation of the Caenorhabditis elegans longevity protein DAF-16 by insulin/IGF-1 and germline signaling. Nat. Genet. 2001;28:139–145. doi: 10.1038/88850. [DOI] [PubMed] [Google Scholar]
42.Tatu U, Braakman I, Helenius A. Membrane glycoprotein folding, oligomerization and intracellular transport: effects of dithiothreitol in living cells. EMBO J. 1993;12:2151–2157. doi: 10.1002/j.1460-2075.1993.tb05863.x. [DOI] [PMC free article] [PubMed] [Google Scholar]
43.Wufuer R, et al. Distinct roles of Nrf1 and Nrf2 in monitoring the reductive stress response to Dithiothreitol (DTT) Antioxidants. 2022;11:1535. doi: 10.3390/antiox11081535. [DOI] [PMC free article] [PubMed] [Google Scholar]
44.Jan CH, Friedman RC, Ruby JG, Bartel DP. Formation, regulation and evolution of Caenorhabditis elegans 3′UTRs. Nature. 2011;469:97–101. doi: 10.1038/nature09616. [DOI] [PMC free article] [PubMed] [Google Scholar]
45.Zisoulis DG, et al. Comprehensive discovery of endogenous Argonaute binding sites in Caenorhabditis elegans. Nat. Struct. Mol. Biol. 2010;17:173–179. doi: 10.1038/nsmb.1745. [DOI] [PMC free article] [PubMed] [Google Scholar]
46.Kuleshov MV, et al. Enrichr: a comprehensive gene set enrichment analysis web server 2016 update. Nucleic Acids Res. 2016;44:W90–W97. doi: 10.1093/nar/gkw377. [DOI] [PMC free article] [PubMed] [Google Scholar]
47.Mori MA, et al. Role of microRNA processing in adipose tissue in stress defense and longevity. Cell Metab. 2012;16:336–347. doi: 10.1016/j.cmet.2012.07.017. [DOI] [PMC free article] [PubMed] [Google Scholar]
48.O’Carroll D, et al. A Slicer-independent role for Argonaute 2 in hematopoiesis and the microRNA pathway. Genes Dev. 2007;21:1999–2004. doi: 10.1101/gad.1565607. [DOI] [PMC free article] [PubMed] [Google Scholar]
49.Reichholf B, et al. Time-resolved small RNA sequencing unravels the molecular principles of microRNA homeostasis. Mol. Cell. 2019;75:756–768.e7. doi: 10.1016/j.molcel.2019.06.018. [DOI] [PMC free article] [PubMed] [Google Scholar]
50.Lee SS, Kennedy S, Tolonen AC, Ruvkun G. DAF-16 target genes that control C. elegans life-span and metabolism. Science. 2003;300:644–647. doi: 10.1126/science.1083614. [DOI] [PubMed] [Google Scholar]
51.Murphy CT, et al. Genes that act downstream of DAF-16 to influence the lifespan of Caenorhabditis elegans. Nature. 2003;424:277–283. doi: 10.1038/nature01789. [DOI] [PubMed] [Google Scholar]
52.Hsin H, Kenyon C. Signals from the reproductive system regulate the lifespan of C. elegans. Nature. 1999;399:362–366. doi: 10.1038/20694. [DOI] [PubMed] [Google Scholar]
53.Berman JR, Kenyon C. Germ-cell loss extends C. elegans life span through regulation of DAF-16 by kri-1 and Lipophilic-hormone signaling. Cell. 2006;124:1055–1068. doi: 10.1016/j.cell.2006.01.039. [DOI] [PubMed] [Google Scholar]
54.Kenyon C, Chang J, Gensch E, Rudner A, Tabtiang R. A C. elegans mutant that lives twice as long as wild type. Nature. 1993;366:461–464. doi: 10.1038/366461a0. [DOI] [PubMed] [Google Scholar]
55.Uno M, et al. A fasting-responsive signaling pathway that extends life span in C. elegans. Cell Rep. 2013;3:79–91. doi: 10.1016/j.celrep.2012.12.018. [DOI] [PubMed] [Google Scholar]
56.De-Souza EA, et al. RNA interference may result in unexpected phenotypes in Caenorhabditis elegans. Nucleic Acids Res. 2019;47:3957–3969. doi: 10.1093/nar/gkz154. [DOI] [PMC free article] [PubMed] [Google Scholar]
57.Jeong H, et al. Deficiency in RCAT-1 function causes dopamine metabolism related behavioral disorders in Caenorhabditis elegans. Int. J. Mol. Sci. 2022;23:2393. doi: 10.3390/ijms23042393. [DOI] [PMC free article] [PubMed] [Google Scholar]
58.Brown KC, Svendsen JM, Tucci RM, Montgomery BE, Montgomery TA. ALG-5 is a miRNA-associated Argonaute required for proper developmental timing in the Caenorhabditis elegans germline. Nucleic Acids Res. 2017;45:9093–9107. doi: 10.1093/nar/gkx536. [DOI] [PMC free article] [PubMed] [Google Scholar]
59.Kirkwood TBL. Evolution of ageing. Mech. Ageing Dev. 2002;123:737–745. doi: 10.1016/S0047-6374(01)00419-5. [DOI] [PubMed] [Google Scholar]
60.Shatalin K, et al. Bacillus anthracis -derived nitric oxide is essential for pathogen virulence and survival in macrophages. Proc. Natl Acad. Sci. 2008;105:1009–1013. doi: 10.1073/pnas.0710950105. [DOI] [PMC free article] [PubMed] [Google Scholar]
61.Amrit FRG, et al. DAF-16 and TCER-1 facilitate adaptation to germline loss by restoring lipid homeostasis and repressing reproductive physiology in C. elegans. PLoS Genet. 2016;12:e1005788. doi: 10.1371/journal.pgen.1005788. [DOI] [PMC free article] [PubMed] [Google Scholar]
62.Pandit A, Jain V, Kumar N, Mukhopadhyay A. PHA-4/FOXA-regulated microRNA feed forward loops during Caenorhabditis elegans dietary restriction. Aging. 2014;6:835–851. doi: 10.18632/aging.100697. [DOI] [PMC free article] [PubMed] [Google Scholar]
63.Schreiner WP, et al. Remodeling of the Caenorhabditis elegans non-coding RNA transcriptome by heat shock. Nucleic Acids Res. 2019;47:9829–9841. doi: 10.1093/nar/gkz693. [DOI] [PMC free article] [PubMed] [Google Scholar]
64.Xu, Y., He, Z., Song, M., Zhou, Y. & Shen, Y. A microRNA switch controls dietary restriction‐induced longevity through Wnt signaling. EMBO Rep.20, e46888 (2019). [DOI] [PMC free article] [PubMed]
65.Guo T, et al. The C. elegans miR-235 regulates the toxicity of graphene oxide via targeting the nuclear hormone receptor DAF-12 in the intestine. Sci. Rep. 2020;10:16933. doi: 10.1038/s41598-020-73712-x. [DOI] [PMC free article] [PubMed] [Google Scholar]
66.Laurindo FRM, Pescatore LA, de Castro Fernandes D. Protein disulfide isomerase in redox cell signaling and homeostasis. Free Radic. Biol. Med. 2012;52:1954–1969. doi: 10.1016/j.freeradbiomed.2012.02.037. [DOI] [PubMed] [Google Scholar]
67.Sies H. Oxidative eustress: On constant alert for redox homeostasis. Redox Biol. 2021;41:101867. doi: 10.1016/j.redox.2021.101867. [DOI] [PMC free article] [PubMed] [Google Scholar]
68.Eletto D, Chevet E, Argon Y, Appenzeller-Herzog C. Redox controls UPR to control redox. J. Cell Sci. 2014;127:3649–3658. doi: 10.1242/jcs.153643. [DOI] [PubMed] [Google Scholar]
69.Feleciano DR, Arnsburg K, Kirstein J. Interplay between redox and protein homeostasis. Worm. 2016;5:e1170273. doi: 10.1080/21624054.2016.1170273. [DOI] [PMC free article] [PubMed] [Google Scholar]
70.Winter AD, McCormack G, Page AP. Protein disulfide isomerase activity is essential for viability and extracellular matrix formation in the nematode Caenorhabditis elegans. Dev. Biol. 2007;308:449–461. doi: 10.1016/j.ydbio.2007.05.041. [DOI] [PubMed] [Google Scholar]
71.Timmons L, Court DL, Fire A. Ingestion of bacterially expressed dsRNAs can produce specific and potent genetic interference in Caenorhabditis elegans. Gene. 2001;263:103–112. doi: 10.1016/S0378-1119(00)00579-5. [DOI] [PubMed] [Google Scholar]
72.Camara H, et al. Tissue-specific overexpression of systemic RNA interference components limits lifespan in C. elegans. Gene. 2024;895:148014. doi: 10.1016/j.gene.2023.148014. [DOI] [PubMed] [Google Scholar]
73.Brosnan CA, Palmer AJ, Zuryn S. Cell-type-specific profiling of loaded miRNAs from Caenorhabditis elegans reveals spatial and temporal flexibility in Argonaute loading. Nat. Commun. 2021;12:1–16. doi: 10.1038/s41467-021-22503-7. [DOI] [PMC free article] [PubMed] [Google Scholar]
74.Chmielarz P, et al. Dicer and microRNAs protect adult dopamine neurons. Cell Death Dis. 2017;8:e2813–e2813. doi: 10.1038/cddis.2017.214. [DOI] [PMC free article] [PubMed] [Google Scholar]
75.Emde A, et al. Dysregulated miRNA biogenesis downstream of cellular stress and ALS‐causing mutations: a new mechanism for ALS. EMBO J. 2015;34:2633–2651. doi: 10.15252/embj.201490493. [DOI] [PMC free article] [PubMed] [Google Scholar]
76.Wei Y, et al. Dicer in macrophages prevents atherosclerosis by promoting mitochondrial oxidative metabolism. Circulation. 2018;138:2007–2020. doi: 10.1161/CIRCULATIONAHA.117.031589. [DOI] [PubMed] [Google Scholar]
77.Schalk A, et al. De novo coding variants in the AGO1 gene cause a neurodevelopmental disorder with intellectual disability. J. Med. Genet. 2022;59:965–975. doi: 10.1136/jmedgenet-2021-107751. [DOI] [PMC free article] [PubMed] [Google Scholar]
78.Lessel D, et al. Germline AGO2 mutations impair RNA interference and human neurological development. Nat. Commun. 2020;11:5797. doi: 10.1038/s41467-020-19572-5. [DOI] [PMC free article] [PubMed] [Google Scholar]
79.Kim MS, et al. Somatic mutations and losses of expression of microRNA regulation-related genes AGO2 and TNRC6A in gastric and colorectal cancers. J. Pathol. 2010;221:139–146. doi: 10.1002/path.2683. [DOI] [PubMed] [Google Scholar]
80.Pinto S, et al. Enoxacin extends lifespan of C. elegans by inhibiting miR-34-5p and promoting mitohormesis. Redox Biol. 2018;18:84–92. doi: 10.1016/j.redox.2018.06.006. [DOI] [PMC free article] [PubMed] [Google Scholar]
81.Yang W, Dierking K, Schulenburg H. WormExp: a web-based application for a Caenorhabditis elegans -specific gene expression enrichment analysis. Bioinformatics. 2016;32:943–945. doi: 10.1093/bioinformatics/btv667. [DOI] [PubMed] [Google Scholar]

Associated Data

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Supplementary Materials

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Description of Additional Supplementary Files

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Supplementary Data 3^{(26.3KB, xlsx)}

Supplementary Data 4^{(126.5KB, xlsx)}

Reporting Summary^{(2.1MB, pdf)}

Source Data^{(1.3MB, xlsx)}

Data Availability Statement

[CR1] 1.López-Otín C, Blasco MA, Partridge L, Serrano M, Kroemer G. Hallmarks of aging: An expanding universe. Cell. 2023;186:243–278. doi: 10.1016/j.cell.2022.11.001. [DOI] [PubMed] [Google Scholar]

[CR2] 2.Pomatto LCD, Davies KJA. The role of declining adaptive homeostasis in ageing. J. Physiol. 2017;595:7275–7309. doi: 10.1113/JP275072. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR3] 3.Blackwell TK, Steinbaugh MJ, Hourihan JM, Ewald CY, Isik M. SKN-1/Nrf, stress responses, and aging in Caenorhabditis elegans. Free Radic. Biol. Med. 2015;88:290–301. doi: 10.1016/j.freeradbiomed.2015.06.008. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR4] 4.Kenyon CJ. The genetics of ageing. Nature. 2010;464:504–512. doi: 10.1038/nature08980. [DOI] [PubMed] [Google Scholar]

[CR5] 5.Bartel DP. Metazoan MicroRNAs. Cell. 2018;173:20–51. doi: 10.1016/j.cell.2018.03.006. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR6] 6.Boehm M, Slack F. A developmental timing MicroRNA and its target regulate life span in C. elegans. Science. 2005;310:1954–1957. doi: 10.1126/science.1115596. [DOI] [PubMed] [Google Scholar]

[CR7] 7.Elder CR, Pasquinelli AE. New roles for MicroRNAs in old worms. Front. Aging. 2022;3:871226. doi: 10.3389/fragi.2022.871226. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR8] 8.de Lencastre A, et al. MicroRNAs both promote and antagonize longevity in C. elegans. Curr. Biol. 2010;20:2159–2168. doi: 10.1016/j.cub.2010.11.015. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR9] 9.Boulias K, Horvitz HR. The C. elegans MicroRNA mir-71 Acts in Neurons to Promote Germline-Mediated Longevity through Regulation of DAF-16/FOXO. Cell Metab. 2012;15:439–450. doi: 10.1016/j.cmet.2012.02.014. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR10] 10.Finger F, et al. Olfaction regulates organismal proteostasis and longevity via microRNA-dependent signalling. Nat .Metab. 2019;1:350–359. doi: 10.1038/s42255-019-0033-z. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR11] 11.Wei Y, Kenyon C. Roles for ROS and hydrogen sulfide in the longevity response to germline loss in Caenorhabditis elegans. Proc. Natl Acad. Sci. 2016;113:E2832–E2841. doi: 10.1073/pnas.1524727113. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR12] 12.Arantes-Oliveira N, Apfeld J, Dillin A, Kenyon C. Regulation of life-span by germ-line stem cells in Caenorhabditis elegans. Science. 2002;295:502–505. doi: 10.1126/science.1065768. [DOI] [PubMed] [Google Scholar]

[CR13] 13.Steinbaugh MJ, et al. Lipid-mediated regulation of SKN-1/Nrf in response to germ cell absence. Elife. 2015;4:e07836. doi: 10.7554/eLife.07836. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR14] 14.Youngman EM, Claycomb JM. From early lessons to new frontiers: the worm as a treasure trove of small RNA biology. Front. Genet. 2014;5:416. doi: 10.3389/fgene.2014.00416. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR15] 15.Zinovyeva AY, Bouasker S, Simard MJ, Hammell CM, Ambros V. Mutations in conserved residues of the C. elegans microRNA Argonaute ALG-1 identify separable functions in ALG-1 miRISC loading and target repression. PLoS Genet. 2014;10:e1004286. doi: 10.1371/journal.pgen.1004286. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR16] 16.Grishok A, et al. Genes and mechanisms related to RNA interference regulate expression of the small temporal RNAs that Control C. elegans developmental timing. Cell. 2001;106:23–34. doi: 10.1016/S0092-8674(01)00431-7. [DOI] [PubMed] [Google Scholar]

[CR17] 17.Aalto AP, et al. Opposing roles of microRNA Argonautes during Caenorhabditis elegans aging. PLoS Genet. 2018;14:e1007379. doi: 10.1371/journal.pgen.1007379. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR18] 18.Finger, F., Ottens, F. & Hoppe, T. The Argonaute Proteins ALG-1 and ALG-2 Are Linked to stress resistance and proteostasis. MicroPubl. Biol. v.2021, 10.17912/micropub.biology.000457 (2021). [DOI] [PMC free article] [PubMed]

[CR19] 19.Pagliuso DC, Bodas DM, Pasquinelli AE. Recovery from heat shock requires the microRNA pathway in Caenorhabditis elegans. PLoS Genet. 2021;17:e1009734. doi: 10.1371/journal.pgen.1009734. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR20] 20.Bukhari SIA, et al. The microRNA pathway controls germ cell proliferation and differentiation in C. elegans. Cell Res. 2012;22:1034–1045. doi: 10.1038/cr.2012.31. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR21] 21.Inukai S, Pincus Z, De Lencastre A, Slack FJ. A microRNA feedback loop regulates global microRNA abundance during aging. RNA. 2018;24:159–172. doi: 10.1261/rna.062190.117. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR22] 22.Kato M, Chen X, Inukai S, Zhao H, Slack FJ. Age-associated changes in expression of small, noncoding RNAs, including microRNAs, in C. elegans. RNA. 2011;17:1804–1820. doi: 10.1261/rna.2714411. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR23] 23.Dutta, S. et al. Efficacy of longevity interventions in C. elegans is determined by early life activity of RNA splicing factors. bioRxiv 2021.11.01.466772 10.1101/2021.11.01.466772 (2021).

[CR24] 24.Gerstein MB, et al. Integrative Analysis of the Caenorhabditis elegans Genome by the modENCODE Project. Science. 2010;330:1775–1787. doi: 10.1126/science.1196914. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR25] 25.Chan S-P, Slack FJ. Ribosomal protein RPS-14 modulates let-7 microRNA function in Caenorhabditis elegans. Dev. Biol. 2009;334:152–160. doi: 10.1016/j.ydbio.2009.07.011. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR26] 26.Lagido C, Pettitt J, Flett A, Glover LA. Bridging the phenotypic gap: real-time assessment of mitochondrial function and metabolism of the nematode Caenorhabditis elegans. BMC Physiol. 2008;8:7. doi: 10.1186/1472-6793-8-7. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR27] 27.Pasquinelli AE, Ruvkun G. Control of Developmental Timing by MicroRNAs and Their Targets. Annu. Rev. Cell Dev. Biol. 2002;18:495–513. doi: 10.1146/annurev.cellbio.18.012502.105832. [DOI] [PubMed] [Google Scholar]

[CR28] 28.Lagos-Quintana M, Rauhut R, Lendeckel W, Tuschl T. Identification of novel genes coding for small expressed RNAs. Science. 2001;294:853–858. doi: 10.1126/science.1064921. [DOI] [PubMed] [Google Scholar]

[CR29] 29.Lau NC, Lim LP, Weinstein EG, Bartel DP. An abundant class of tiny RNAs with probable regulatory roles in Caenorhabditis elegans. Science. 2001;294:858–862. doi: 10.1126/science.1065062. [DOI] [PubMed] [Google Scholar]

[CR30] 30.Seth P, et al. Regulation of MicroRNA machinery and development by interspecies S-Nitrosylation. Cell. 2019;176:1014–1025.e12. doi: 10.1016/j.cell.2019.01.037. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR31] 31.Bito T, et al. Vitamin B12 deficiency results in severe oxidative stress, leading to memory retention impairment in Caenorhabditis elegans. Redox Biol. 2017;11:21–29. doi: 10.1016/j.redox.2016.10.013. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR32] 32.Gusarov I, et al. Bacterial nitric oxide extends the lifespan of C. elegans. Cell. 2013;152:818–830. doi: 10.1016/j.cell.2012.12.043. [DOI] [PubMed] [Google Scholar]

[CR33] 33.Hao Y, et al. Thioredoxin shapes the C. elegans sensory response to Pseudomonas produced nitric oxide. Elife. 2018;7:e36833. doi: 10.7554/eLife.36833. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR34] 34.Piacenza L, Zeida A, Trujillo M, Radi R. The superoxide radical switch in the biology of nitric oxide and peroxynitrite. Physiol. Rev. 2022;102:1881–1906. doi: 10.1152/physrev.00005.2022. [DOI] [PubMed] [Google Scholar]

[CR35] 35.Radi R. Oxygen radicals, nitric oxide, and peroxynitrite: Redox pathways in molecular medicine. Proc. Natl Acad. Sci. 2018;115:5839–5848. doi: 10.1073/pnas.1804932115. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR36] 36.Bus JS, Gibson JE. Paraquat: model for oxidant-initiated toxicity. Environ. Health Perspect. 1984;55:37–46. doi: 10.1289/ehp.845537. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR37] 37.Bagley AC, Krall J, Lynch RE. Superoxide mediates the toxicity of paraquat for Chinese hamster ovary cells. Proc. Natl Acad. Sci. 1986;83:3189–3193. doi: 10.1073/pnas.83.10.3189. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR38] 38.Guidarelli A, Fiorani M, Cerioni L, Cantoni O. The compartmentalised nature of the mechanisms governing superoxide formation and scavenging in cells exposed to arsenite. Toxicol. Appl. Pharmacol. 2019;384:114766. doi: 10.1016/j.taap.2019.114766. [DOI] [PubMed] [Google Scholar]

[CR39] 39.An JH, Blackwell TK. SKN-1 links C. elegans mesendodermal specification to a conserved oxidative stress response. Genes Dev. 2003;17:1882–1893. doi: 10.1101/gad.1107803. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR40] 40.Yamawaki TM, Arantes-Oliveira N, Berman JR, Zhang P, Kenyon C. Distinct activities of the germline and somatic reproductive tissues in the regulation of Caenorhabditis elegans’ longevity. Genetics. 2008;178:513–526. doi: 10.1534/genetics.107.083253. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR41] 41.Lin K, Hsin H, Libina N, Kenyon C. Regulation of the Caenorhabditis elegans longevity protein DAF-16 by insulin/IGF-1 and germline signaling. Nat. Genet. 2001;28:139–145. doi: 10.1038/88850. [DOI] [PubMed] [Google Scholar]

[CR42] 42.Tatu U, Braakman I, Helenius A. Membrane glycoprotein folding, oligomerization and intracellular transport: effects of dithiothreitol in living cells. EMBO J. 1993;12:2151–2157. doi: 10.1002/j.1460-2075.1993.tb05863.x. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR43] 43.Wufuer R, et al. Distinct roles of Nrf1 and Nrf2 in monitoring the reductive stress response to Dithiothreitol (DTT) Antioxidants. 2022;11:1535. doi: 10.3390/antiox11081535. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR44] 44.Jan CH, Friedman RC, Ruby JG, Bartel DP. Formation, regulation and evolution of Caenorhabditis elegans 3′UTRs. Nature. 2011;469:97–101. doi: 10.1038/nature09616. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR45] 45.Zisoulis DG, et al. Comprehensive discovery of endogenous Argonaute binding sites in Caenorhabditis elegans. Nat. Struct. Mol. Biol. 2010;17:173–179. doi: 10.1038/nsmb.1745. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR46] 46.Kuleshov MV, et al. Enrichr: a comprehensive gene set enrichment analysis web server 2016 update. Nucleic Acids Res. 2016;44:W90–W97. doi: 10.1093/nar/gkw377. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR47] 47.Mori MA, et al. Role of microRNA processing in adipose tissue in stress defense and longevity. Cell Metab. 2012;16:336–347. doi: 10.1016/j.cmet.2012.07.017. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR48] 48.O’Carroll D, et al. A Slicer-independent role for Argonaute 2 in hematopoiesis and the microRNA pathway. Genes Dev. 2007;21:1999–2004. doi: 10.1101/gad.1565607. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR49] 49.Reichholf B, et al. Time-resolved small RNA sequencing unravels the molecular principles of microRNA homeostasis. Mol. Cell. 2019;75:756–768.e7. doi: 10.1016/j.molcel.2019.06.018. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR50] 50.Lee SS, Kennedy S, Tolonen AC, Ruvkun G. DAF-16 target genes that control C. elegans life-span and metabolism. Science. 2003;300:644–647. doi: 10.1126/science.1083614. [DOI] [PubMed] [Google Scholar]

[CR51] 51.Murphy CT, et al. Genes that act downstream of DAF-16 to influence the lifespan of Caenorhabditis elegans. Nature. 2003;424:277–283. doi: 10.1038/nature01789. [DOI] [PubMed] [Google Scholar]

[CR52] 52.Hsin H, Kenyon C. Signals from the reproductive system regulate the lifespan of C. elegans. Nature. 1999;399:362–366. doi: 10.1038/20694. [DOI] [PubMed] [Google Scholar]

[CR53] 53.Berman JR, Kenyon C. Germ-cell loss extends C. elegans life span through regulation of DAF-16 by kri-1 and Lipophilic-hormone signaling. Cell. 2006;124:1055–1068. doi: 10.1016/j.cell.2006.01.039. [DOI] [PubMed] [Google Scholar]

[CR54] 54.Kenyon C, Chang J, Gensch E, Rudner A, Tabtiang R. A C. elegans mutant that lives twice as long as wild type. Nature. 1993;366:461–464. doi: 10.1038/366461a0. [DOI] [PubMed] [Google Scholar]

[CR55] 55.Uno M, et al. A fasting-responsive signaling pathway that extends life span in C. elegans. Cell Rep. 2013;3:79–91. doi: 10.1016/j.celrep.2012.12.018. [DOI] [PubMed] [Google Scholar]

[CR56] 56.De-Souza EA, et al. RNA interference may result in unexpected phenotypes in Caenorhabditis elegans. Nucleic Acids Res. 2019;47:3957–3969. doi: 10.1093/nar/gkz154. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR57] 57.Jeong H, et al. Deficiency in RCAT-1 function causes dopamine metabolism related behavioral disorders in Caenorhabditis elegans. Int. J. Mol. Sci. 2022;23:2393. doi: 10.3390/ijms23042393. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR58] 58.Brown KC, Svendsen JM, Tucci RM, Montgomery BE, Montgomery TA. ALG-5 is a miRNA-associated Argonaute required for proper developmental timing in the Caenorhabditis elegans germline. Nucleic Acids Res. 2017;45:9093–9107. doi: 10.1093/nar/gkx536. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR59] 59.Kirkwood TBL. Evolution of ageing. Mech. Ageing Dev. 2002;123:737–745. doi: 10.1016/S0047-6374(01)00419-5. [DOI] [PubMed] [Google Scholar]

[CR60] 60.Shatalin K, et al. Bacillus anthracis -derived nitric oxide is essential for pathogen virulence and survival in macrophages. Proc. Natl Acad. Sci. 2008;105:1009–1013. doi: 10.1073/pnas.0710950105. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR61] 61.Amrit FRG, et al. DAF-16 and TCER-1 facilitate adaptation to germline loss by restoring lipid homeostasis and repressing reproductive physiology in C. elegans. PLoS Genet. 2016;12:e1005788. doi: 10.1371/journal.pgen.1005788. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR62] 62.Pandit A, Jain V, Kumar N, Mukhopadhyay A. PHA-4/FOXA-regulated microRNA feed forward loops during Caenorhabditis elegans dietary restriction. Aging. 2014;6:835–851. doi: 10.18632/aging.100697. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR63] 63.Schreiner WP, et al. Remodeling of the Caenorhabditis elegans non-coding RNA transcriptome by heat shock. Nucleic Acids Res. 2019;47:9829–9841. doi: 10.1093/nar/gkz693. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR64] 64.Xu, Y., He, Z., Song, M., Zhou, Y. & Shen, Y. A microRNA switch controls dietary restriction‐induced longevity through Wnt signaling. EMBO Rep.20, e46888 (2019). [DOI] [PMC free article] [PubMed]

[CR65] 65.Guo T, et al. The C. elegans miR-235 regulates the toxicity of graphene oxide via targeting the nuclear hormone receptor DAF-12 in the intestine. Sci. Rep. 2020;10:16933. doi: 10.1038/s41598-020-73712-x. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR66] 66.Laurindo FRM, Pescatore LA, de Castro Fernandes D. Protein disulfide isomerase in redox cell signaling and homeostasis. Free Radic. Biol. Med. 2012;52:1954–1969. doi: 10.1016/j.freeradbiomed.2012.02.037. [DOI] [PubMed] [Google Scholar]

[CR67] 67.Sies H. Oxidative eustress: On constant alert for redox homeostasis. Redox Biol. 2021;41:101867. doi: 10.1016/j.redox.2021.101867. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR68] 68.Eletto D, Chevet E, Argon Y, Appenzeller-Herzog C. Redox controls UPR to control redox. J. Cell Sci. 2014;127:3649–3658. doi: 10.1242/jcs.153643. [DOI] [PubMed] [Google Scholar]

[CR69] 69.Feleciano DR, Arnsburg K, Kirstein J. Interplay between redox and protein homeostasis. Worm. 2016;5:e1170273. doi: 10.1080/21624054.2016.1170273. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR70] 70.Winter AD, McCormack G, Page AP. Protein disulfide isomerase activity is essential for viability and extracellular matrix formation in the nematode Caenorhabditis elegans. Dev. Biol. 2007;308:449–461. doi: 10.1016/j.ydbio.2007.05.041. [DOI] [PubMed] [Google Scholar]

[CR71] 71.Timmons L, Court DL, Fire A. Ingestion of bacterially expressed dsRNAs can produce specific and potent genetic interference in Caenorhabditis elegans. Gene. 2001;263:103–112. doi: 10.1016/S0378-1119(00)00579-5. [DOI] [PubMed] [Google Scholar]

[CR72] 72.Camara H, et al. Tissue-specific overexpression of systemic RNA interference components limits lifespan in C. elegans. Gene. 2024;895:148014. doi: 10.1016/j.gene.2023.148014. [DOI] [PubMed] [Google Scholar]

[CR73] 73.Brosnan CA, Palmer AJ, Zuryn S. Cell-type-specific profiling of loaded miRNAs from Caenorhabditis elegans reveals spatial and temporal flexibility in Argonaute loading. Nat. Commun. 2021;12:1–16. doi: 10.1038/s41467-021-22503-7. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR74] 74.Chmielarz P, et al. Dicer and microRNAs protect adult dopamine neurons. Cell Death Dis. 2017;8:e2813–e2813. doi: 10.1038/cddis.2017.214. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR75] 75.Emde A, et al. Dysregulated miRNA biogenesis downstream of cellular stress and ALS‐causing mutations: a new mechanism for ALS. EMBO J. 2015;34:2633–2651. doi: 10.15252/embj.201490493. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR76] 76.Wei Y, et al. Dicer in macrophages prevents atherosclerosis by promoting mitochondrial oxidative metabolism. Circulation. 2018;138:2007–2020. doi: 10.1161/CIRCULATIONAHA.117.031589. [DOI] [PubMed] [Google Scholar]

[CR77] 77.Schalk A, et al. De novo coding variants in the AGO1 gene cause a neurodevelopmental disorder with intellectual disability. J. Med. Genet. 2022;59:965–975. doi: 10.1136/jmedgenet-2021-107751. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR78] 78.Lessel D, et al. Germline AGO2 mutations impair RNA interference and human neurological development. Nat. Commun. 2020;11:5797. doi: 10.1038/s41467-020-19572-5. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR79] 79.Kim MS, et al. Somatic mutations and losses of expression of microRNA regulation-related genes AGO2 and TNRC6A in gastric and colorectal cancers. J. Pathol. 2010;221:139–146. doi: 10.1002/path.2683. [DOI] [PubMed] [Google Scholar]

[CR80] 80.Pinto S, et al. Enoxacin extends lifespan of C. elegans by inhibiting miR-34-5p and promoting mitohormesis. Redox Biol. 2018;18:84–92. doi: 10.1016/j.redox.2018.06.006. [DOI] [PMC free article] [PubMed] [Google Scholar]

[CR81] 81.Yang W, Dierking K, Schulenburg H. WormExp: a web-based application for a Caenorhabditis elegans -specific gene expression enrichment analysis. Bioinformatics. 2016;32:943–945. doi: 10.1093/bioinformatics/btv667. [DOI] [PubMed] [Google Scholar]

PERMALINK

An Intricate Network Involving the Argonaute ALG-1 Modulates Organismal Resistance to Oxidative Stress

Carlos A Vergani-Junior

Raíssa De P Moro

Silas Pinto

Evandro A De-Souza

Henrique Camara

Deisi L Braga

Guilherme Tonon-da-Silva

Thiago L Knittel

Gabriel P Ruiz

Raissa G Ludwig

Katlin B Massirer

William B Mair

Marcelo A Mori

Abstract

Introduction

Results

Loss of alg-1 in adult C. elegans disrupts redox balance

ALG-1 is upregulated in multiple long-lived mutants

Fig. 1. ALG-1 levels are increased in long-lived mutants.

Worms overexpressing ALG-1 are oxidative stress resistant

Fig. 2. alg-1 overexpression improves oxidative stress resistance.

Downregulation of R02D3.7 protects from oxidative stress

Fig. 3. Knockdown of R02D3.7 increases oxidative stress resistance.

miRNAs induced by ALG-1/OE confer oxidative stress resistance

Fig. 4. Increased miRNAs upon ALG-1 overexpression control resistance to oxidative stress.

miRNAs induced by ALG-1/OE target and limit the PDI pathway

Fig. 5. Fine-tuning of the PDI pathway by miRNAs improves oxidative stress resistance.

Fig. 6. An intricate mechanism involving the miRNA biogenesis machinery regulates oxidative stress resistance in C. elegans.

Discussion

Methods

Strains and maintenance of C. elegans

RNAi

Lifespans assays

Oxidative stress induced by sodium arsenite

Mobility analysis

Pharyngeal pumping

Duration of development

Brood size assay

ModENCODE analysis

GFP reporter analyses

Real-time qPCR

Small RNA sequencing

RNAseq data analysis

Gene ontology of miRNA targets

pdi-2 3’UTR cloning

miR-230-3p target assay

Statistics

Reporting summary

Supplementary information

Source data

Acknowledgements

Author contributions

Peer review

Peer review information

Data availability

Competing interests

Footnotes

Supplementary information

References

Associated Data

Supplementary Materials

Data Availability Statement

ACTIONS

PERMALINK

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