Diet is a crucial determinant of organismal biology; interactions between the host, its diet, and its microbiota are critical to determining the health of an organism. A variety of genetic and biochemical means were used to assay stress sensitivity in C. elegans reared on two standard laboratory diets: E. coli OP50, the most commonly used food for C. elegans, or E. coli HT115, which is typically used for RNAi-mediated gene knockdown. We demonstrated that the relatively subtle shift to a diet of E. coli HT115 had a dramatic impact on C. elegans’s survival after exposure to pathogenic or abiotic stresses. Interestingly, this was independent of canonical host defense pathways. Instead the change arises from improvements in mitochondrial health, likely due to alleviation of a vitamin B12 deficiency exhibited by worms reared on an E. coli OP50 diet. Increasing B12 availability, by feeding on E. coli HT115, supplementing E. coli OP50 with exogenous vitamin B12, or overexpression of the B12 transporter, improved mitochondrial homeostasis and increased resistance. Loss of the methylmalonyl-CoA mutase gene mmcm-1/MUT, which requires vitamin B12 as a cofactor, abolished these improvements, establishing a genetic basis for the E. coli OP50-incurred sensitivity. Our study forges a mechanistic link between a dietary deficiency (nutrition/microbiota) and a physiological consequence (host sensitivity), using the host-microbiota-diet framework.
Vitamin B12 deficiency affects ~10–40% of US adults, causing a range of health issues ranging from anemia to neurological defects. Here we provide a mechanistic link between dietary B12 deficiency and mitochondrial dysfunction. Our data indicate that B12 supports clearance of propionate, an intermediate of branched chain amino acid metabolism. Excess propionate compromises mitochondrial homeostasis, increasing susceptibility to abiotic stresses and bacterial pathogenesis. Importantly, this deficiency is absent when worms are fed a diet of E. coli HT115. C. elegans reared on E. coli OP50 are predisposed to a variety of health defects, including increased sensitivity to bacterial pathogens and stresses; these subtle phenotypes may be difficult to recapitulate under conventional RNAi feeding conditions with HT115, introducing unexpected experimental confounds. These findings reinforce the importance of considering the host-microbiota-nutrient axis when using this model organism.
Citation: Revtovich AV, Lee R, Kirienko NV (2019) Interplay between mitochondria and diet mediates pathogen and stress resistance in Caenorhabditis elegans. PLoS Genet 15(3): e1008011. https://doi.org/10.1371/journal.pgen.1008011
Editor: Danielle A. Garsin, The University of Texas Health Science Center at Houston, UNITED STATES
Received: August 17, 2018; Accepted: February 9, 2019; Published: March 13, 2019
Copyright: © 2019 Revtovich et al. This is an open access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Data Availability: Microarray data are available from the GEO database and can be accessed using following link: https://www.ncbi.nlm.nih.gov/geo/query/acc.cgi?token=kjibcyuydrstvuj&acc=GSE97678. All other relevant data are within the paper and its Supporting Information files.
Funding: This study was funded by following grants to NK: K22AI110552 (NIH NIAID), R35GM129294 (NIH NIGMS), RR150044 (Cancer Prevention Research Institute of Texas), and C-1930 (Welch Foundation). The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
Like it's genome, an organism's diet and microbiota tremendously influence its life history. Attempts to understand this have led to the development of the host-microbiota-nutrition axis model . Although an avalanche of literature has reported on variations in the microbiota, diet, and genomes of model organisms, mechanistic understanding has lagged considerably behind description. The dynamic and complex interactions between these three systems form something of a "biological three-body problem". For example, host genetics and microbiotic metabolism influence the nutritional value of the diet consumed [2,3]. Simultaneously, the host's environment determines its initial susceptibility to microbial colonization . Despite the difficulty, it is crucial to establish a mechanistic understanding of these interrelationships to properly understand host healthspan under normal and stress conditions.
Caenorhabditis elegans offers a tantalizing system for simplifying these studies without sacrificing the ability to make discoveries useful for more complex organisms. Generation of gnotobiotic worms is simple, efficient, and inexpensive, only requiring treatment of gravid adults with hypochlorite to release eggs that will hatch into microbe-free larvae. C. elegans can then simply be transferred to agar plates seeded with a wide-variety of bacteria (either a single strain or a customized mixture). Generally, the host readily consumes the bacteria provided. In its most reductionist form, the host-microbiota-nutrition axis of C. elegans can be collapsed to a binary system comprised of only two species, both of which are genetically tractable: C. elegans, the bacterivorous host, and E. coli, which serves as food. Although C. elegans is typically not colonized by E. coli the way that humans are (at least not early in its life), Cabreiro and Gems make a compelling argument that E. coli serves at least most of the functions for C. elegans that a conventional microbiota confers to its host, including protection against pathogens, immune maturation, digestive aid, vitamin production, and xenobiotic metabolism . So by at least some definitions, E. coli can comprise a microbiota for C. elegans as well.
Even this simple binary system has yielded a number of significant insights into the complicated interactions between host, diet, and microbiota. Different diets profoundly affect the worm transcriptome , metabolome , intestinal fat storage  and lifespan [6–9]. The metabolic activity of the bacterial food also influences the metabolism of C. elegans [10,11]. For example, C. elegans feeding on Bacillus subtilis were observed to have a greater lifespan than their E. coli-fed counterparts . This effect was shown to be a consequence of the host utilizing bacterially-derived nitric oxide to stimulate expression of HSF-1 and DAF-16, which increase lifespan . In contrast, C. elegans's lifespan can be shortened by bacterial folate metabolism [14,15], probably via increased S-adenosylmethionine (SAM) synthesis . The link between SAM and lifespan was demonstrated by an elegant study that showed that metformin, by limiting SAM production and stimulating AMPK activation, increases C. elegans lifespan . Unfortunately, this is unlikely to be a viable method to increase healthspan; SAM is a crucial methyl group donor necessary for a wide variety of cellular activities. For example, C. elegans sams-1 (RNAi) mutants exhibit constitutive immune activation, but despite this, they show increased sensitivity to Pseudomonas aeruginosa .
Like humans, C. elegans is incapable of creating several essential vitamins, including vitamin B12, and they must be obtained from their diet. Vitamin B12 exists as two biologically active, readily interconvertible vitamers, methylcobalamin and adenosylcobalamin. These compounds are involved in the biosynthesis of methionine and the conversion of methylmalonyl-CoA to succinyl-CoA, respectively. This latter pathway is required for the proper breakdown of propionate and branched-chain amino acids, the failure of which is associated with mitochondrial dysfunction [18,19]. Serious consequences have been associated with severe vitamin B12 deficiency in C. elegans, including infertility, slowed growth, and shortened lifespan [20,21]. In both C. elegans and mammals, B12 deficiency causes toxic intermediates to accumulate [22,23]. Interestingly, the most common C. elegans lab diet, E. coli OP50, results in a mild, chronic vitamin B12 deficiency [6,21].
Through a variety of assays, we discovered that the vitamin B12 deficiency caused by a diet of E. coli strain OP50 disrupts mitochondrial homeostasis, sensitizing the host to infection and a variety of abiotic stresses. B12 supplementation, even in the absence of living bacteria, increased resistance without affecting lifespan. Genetic analysis mapped this phenotype to the methylmalonyl/succinyl-CoA breakdown pathway, where vitamin B12 serves as a cofactor for MMCM-1/MUT. Our findings provide a mechanistic link between diet, cellular homeostasis, and organismal health.
A diet of E. coli strain HT115 confers resistance to multiple bacterial pathogens
While characterizing a C. elegans-P. aeruginosa Liquid Killing assay [24,25], we made the unexpected observation that diet plays a large role in the hosts' survival after exposure to P. aeruginosa strain PA14. For example, median survival time of glp-4(bn2) worms reared on E. coli HT115 was 48h, while worms reared on E. coli OP50 showed median survival closer to 30h (Fig 1A and 1B). E. coli HT115 is used ubiquitously for RNAi in C. elegans; this strain is the host for the two largest, publicly available whole-genome RNAi libraries [26,27]. Importantly, the increase in resistance to P. aeruginosa PA14 occurred regardless of whether either E. coli strain carried the L4440 RNAi plasmid vector (S1A Fig). Pathogenesis in this assay depends on intoxication with the siderophore pyoverdine, which removes iron from the C. elegans host [28,29]. 1,10-phenanthroline, a small synthetic chelator, mimics many of the aspects of siderophore-mediated killing [29,30], so resistance of E. coli HT115-fed worms to this compound was also assayed. glp-4(bn2) worms fed HT115 were more resistant to phenanthroline than their OP50-fed counterparts (Fig 1C).
(A) Representative bright-field (top) and fluorescent (bottom) images of glp-4(bn2) C. elegans exposed to P. aeruginosa PA14 after feeding on E. coli OP50 or E. coli HT115. Fraction of surviving worms (here and elsewhere) was inferred based on staining with Sytox Orange, a cell impermeant dye. (B) Time course of Liquid Killing of C. elegans as in (A). (C-G) Survival of OP50- and HT115-fed glp-4(bn2) worms after acute phenanthroline poisoning (100 μM) (C), infection with E. faecalis OG1RF (D), or exposure to hyperthermic (30°C) (E) or oxidative stresses from juglone (120 μM) (F) or hydrogen peroxide (2 mM) (G). (H) Lifespan of C. elegans fed with E. coli OP50 or E. coli HT115. p-value for (B-G) <0.01, (H) > 0.05 (N.S.). p-values were calculated using log-rank test (B,C,E,F,H) or Student’s t-test (D,G). *—p<0.01. At least 10 wells, each containing 20 worms, were used per replicate for (A,B,D,G). At least 50 worms per plate, three plates per condition per replicate were used for (C,E,F,H). At least three biological replicates were performed for each experiment.
We have previously shown that exogenous iron strongly limited the ability of pyoverdine or 1,10-phenanthroline to cause host death . Therefore, one possibility is that E. coli HT115 may be indirectly increasing resistance by providing more iron to C. elegans. To test this hypothesis, total host iron, using inductively-coupled plasma mass spectrometry, or iron (III), using a fluorometric method, were measured. In each assay, iron levels were indistinguishable, regardless of the food tested (S1B and S1C Fig).
Since these findings suggested that the deficiency was not related to iron, we suspected the sensitivity may also exist for other pathogens. To test this, glp-4(bn2) worms were reared on either E. coli OP50 or HT115, and then exposed to Enterococcus faecalis OG1RF, another human bacterial pathogen, in a recently-developed Liquid Killing assay . To the best of our knowledge, pathogenesis in this assay is independent of siderophores. Interestingly, E. coli HT115 also increased survival of C. elegans infected with this pathogen by ~30% (Fig 1D). E. faecalis OG1RF is a gram positive pathogen that likely uses different pathogenic determinants than P. aeruginosa PA14 , suggesting that the mechanism of resistance has a broad spectrum of activity.
The ability of E. coli HT115 to confer resistance to P. aeruginosa-mediated slow killing was also tested. Unlike the liquid-based pathogenesis assays, no statistically significant difference was seen between worms reared on the two diets (S2A Fig). To ensure that the worms were not colonized differently, a strain of P. aeruginosa engineered to express DsRed was used to infect worms after they were reared on each diet. Again, no statistically significant difference was observed (S2B and S2C Fig). One possible explanation for this difference is that pathogenesis in this assay is thought to take place via intestinal colonization; the biological difference induced by a diet of E. coli HT115 may be irrelevant for this mechanism of pathogenesis.
Diet-mediated sensitivity is independent of innate immunity
Substitution of E. coli OP50 with a variety of other bacterial foods (or dead E. coli) increases the lifespan of C. elegans [33–36]. This is often interpreted as evidence that E. coli OP50 is weakly pathogenic to C. elegans [37,38], opening the possibility that E. coli HT115 is less pathogenic than E. coli OP50 (at least under these conditions). In this case, it is likely that the immune response of C. elegans would differ between OP50 and HT115. Transcription of a number of C. elegans innate immune genes, regulated by PMK-1/p38, ZIP-2/bZIP, DAF-16/FOXO, FSHR-1/FSH, and SKN-1/Nrf [12,39–43] was surveyed. Synchronized glp-4(bn2) worms were reared on either E. coli OP50 or E. coli HT115 to the young adult stage and basal gene expression for these pathways was assessed. Gene expression levels were indistinguishable between food sources (S3 Fig).
We also assayed induction, rather than basal expression, of the innate immune pathways using RNAi. As noted above, RNAi in C. elegans is typically performed using E. coli HT115, in part because E. coli OP50 generally expresses dsRNA quite poorly . Fortunately, an RNAseIII-deficient strain of OP50, called xu363, that efficiently produce dsRNA at levels comparable to E. coli HT115 has recently been engineered . Comparisons of cyc-1(RNAi) in the two strains (E. coli OP50(xu363) and E. coli HT115) suggest that they exhibit comparable levels of gene knockdown (S4 Fig).
RNAi constructs for pmk-1, zip-2, daf-16, fshr-1, and skn-1 were transferred from E. coli HT115 into E. coli OP50(xu363). glp-4(bn2) mutants were then reared on either E. coli OP50(xu363) or E. coli HT115 expressing each RNAi construct. At the young adult stage, pathogenesis in the Liquid Killing assay was tested. As expected, some gene disruptions altered the timing of death compared to bacteria containing an empty RNAi vector. For example, daf-16 knockdown, which sensitizes worms to Liquid Killing , hastened death in each case. daf-2(RNAi), which constitutively activates DAF-16/FOXO, prolonged survival. Importantly, worms fed E. coli HT115 survived longer than worms fed E. coli OP50(xu363), regardless of the gene targeted by RNAi (S5 Fig). Combined, these data indicate that the weak pathogenicity reported for E. coli OP50 is unlikely to be causing the increased sensitivity to P. aeruginosa, phenanthroline, and E. faecalis.
E. coli HT115 also promotes resistance to abiotic stresses
Several innate immune pathways in C. elegans (such as those regulated by DAF-16/FOXO, SKN-1/Nrf, or the ESRE network) also promote survival during exposure to abiotic stresses, like heat or free-radical inducing chemicals. glp-4(bn2) worms were reared on E. coli OP50 or E. coli HT115 and then exposed as young adult worms to either heat shock, juglone, or hydrogen peroxide. In each case, E. coli HT115-fed worms survived better (Fig 1E–1G). Because increased stress or pathogen resistance is often associated with longer lifespan (which has led to the theory that the former is responsible for the latter), we compared the average lifespan of worms reared on these bacteria. However, E. coli HT115 did not increase host lifespan (Fig 1H).
Increased resistance is not due to the glp-4(bn2) phenotype
Another possible explanation that emerged was the temperature-dependent sterility induced by the glp-4(bn2) phenotype. For technical reasons, it is necessary to induce sterility in worms for liquid-based killing assays . The glp-4(bn2) mutation compromises a valyl aminoacyl tRNA synthetase (VARS-2)  which prevents development of the germline, but causes no other overt phenotype [47–49]. When the germline of C. elegans is removed, lifespan is extended in a DAF-16/FOXO-dependent fashion [50,51]. Since this transcription factor promotes broad-spectrum stress resistance, it was important to determine whether wild-type C. elegans also exhibited a difference in stress resistance when reared on E. coli HT115.
Wild-type N2 worms were reared on E. coli OP50 or E. coli HT115 and then subjected to Liquid Killing, propionate, or heat shock. Lifespans were also measured. In each case, results from wild-type worms recapitulated our findings from glp-4(bn2) mutants (S6 Fig).
Transcriptome profiling implicates mitochondrial perturbations in OP50-induced stress sensitivity
Without a clear explanation for the diet-induced difference in stress resistance, we turned toward microarray analysis to get an unbiased representation of transcriptional events. glp-4(bn2) worms were reared to young adult stage on either E. coli OP50 or E. coli HT115. RNA was collected and microarray analysis was performed essentially as previously described . To our surprise, the number of genes differentially regulated was relatively small; only 35 genes showed upregulation between 2- and 8-fold in E. coli HT115, while 22 genes were upregulated (between 2- and 20-fold) in E. coli OP50 (Fig 2A, S1 Table). Interestingly, 12 of the latter 22 genes encode proteins predicted to be localized to the mitochondria (Table 1).
(A) Number of genes upregulated in worms fed either E. coli HT115 or E. coli OP50 when normalized to the other food. Genes annotated as having a mitochondrial localization or function are shown in black, while non-mitochondrial genes are shown in grey. (B) Visualization of acdh-1p::GFP reporter fluorescence in worms fed E. coli OP50 or E. coli HT115, with or without methylcobalamin supplementation (200 ng/ml), as indicated (see S7A Fig for quantification). (C) acdh-1p::GFP expression in worms reared on E. coli OP50 or E. coli HT115 with or without methylcobalamin supplementation was measured using flow vermimetry. Fluorescence for each worm was normalized to its size (see S7B Fig for quantification). (D,E) acdh-1p::GFP fluorescence of worms reared on E. coli OP50 or E. coli HT115 supplemented with varying concentrations of methlycobalamin. (F, G) acdh-1p::GFP fluorescence of worms reared as in (C) with exogenous propionate. (H) Propionate toxicity in worms fed as in (C). *—p<0.01, p-value was calculated based on Student’s t-test. For (C-E) at least 1500 worms were used for each replicate. For (H) approximately 70 worms were used per plate per condition per biological replicate. At least three biological replicates were performed for each experiment.
This enrichment was strongly significant (p = 2.2*10−16), particularly given the small fraction of nuclear genes that encode mitochondrial proteins in C. elegans (~6%) and humans (7%) [52,56]. In contrast, only two genes encoding proteins targeted to the mitochondria (acox-2 and T22B7.7) were upregulated in E. coli HT115 compared to E. coli OP50 (2/35 = 5.7%, p = 0.9896). Of the genes upregulated in worms fed E. coli OP50, two caught our attention: hsp-60, which encodes a mitochondrial chaperone upregulated on mitochondrial damage [57,58] and acdh-1, which encodes a short-chain acyl-CoA dehydrogenase that is upregulated when dietary sources are rich in branched-chain amino acids and/or propionyl-CoA, which can be toxic to mitochondria . When these data were compared to a previous study, which used slightly different methodology to determine differentially regulated genes, the results had striking concordance (S2 Table). Overlap between the genes downregulated in each study or upregulated in each study was significant (p-value 1.42*10−11 and 4.97*10−22, respectively). Moreover, 70% of the genes downregulated in both studies are annotated as mitochondrially-localized or have a putative function in mitochondria.
We crossed the acdh-1p::GFP reporter into a glp-4(bn2) background, and then reared the resulting strain on either E. coli OP50 or E. coli HT115. We saw increased expression of acdh-1p::GFP in E. coli OP50-fed worms, whether measured by conventional imaging (Fig 2B, see S7A Fig for quantification) or by flow vermimetry (Fig 2C, see S7B Fig for quantification). Our transcriptome profiling and acdh-1 expression data are in concordance with previous reports, where an E. coli OP50 diet increased expression of acdh-1p::GFP and transcription of several other genes encoding mitochondrially-targeted proteins [22,23]. These traits have been associated with a mild to moderate vitamin B12 deficiency [6,21].
We attempted to use mass spectrometry to quantify adenosylcobalamin in worms fed with either E. coli OP50 or E. coli HT115. We also tried to quantify it in bacterial slurries from each strain. Unfortunately, B12 levels for all samples measured were below the detection threshold of the instrument. Although we were unable to measure precise amounts of vitamin B12 in the host or in the bacteria, qualitative methods are available to test whether E. coli HT115 is a better source of vitamin B12, based on acdh-1p::GFP fluorescence and propionate toxicity. First, the bacterial growth media was spiked with exogenous methylcobalamin to a final concentration of 200 ng/mL, bacteria were grown as usual, and spotted onto NGM media plates. Worms were reared on these plates and then acdh-1p::GFP expression was measured at the young adult stage using flow vermimetry. Vitamin supplementation dramatically reduced acdh-1p::GFP expression (Fig 2C, S7A Fig). The same approach was used, with differing concentrations, to determine the amount of exogenous B12 required to reduce acdh-1p::GFP fluorescence in worms reared on each food. Comparable fluorescence was observed when E. coli OP50 and E. coli HT115 were supplemented with 50 μM and 3.1 μM, respectively (Fig 2D and 2E).
Second, expression of acdh-1p::GFP can be compared when worms are exposed to exogenous propionate [22,23]. Although worms reared on E. coli OP50 consistently showed more fluorescence than worms fed E. coli HT115, adding propionate to media increased acdh-1p::GFP expression regardless of diet (Fig 2F and 2G, see S7B Fig for quantification). For example, fluorescence was similar in worms reared on E. coli OP50 and E. coli HT115 spiked with 25 mM and 50 mM propionate, respectively.
Finally, in addition to triggering acdh-1 expression, excess propionate is toxic to C. elegans [22,23,60]. Vitamin B12 sufficiency is proportional to increased survival. Young adult worms reared on either E. coli OP50 or E. coli HT115 were exposed to varying concentrations of propionate and survival was measured after 24h. Worms reared on E. coli HT115 exhibited increased resistance compared to E. coli OP50, and the addition of methylcobalamin to their diet improved each group further still (Fig 2H). All three assays qualitatively support the conclusion that E. coli HT115 is a better source of vitamin B12 than E. coli OP50, a finding that is consistent with previous reports [6,22,23].
Vitamin B12 supplementation improves mitochondrial health
Because excess propionate is known to cause mitochondrial toxicity [59,61], we assayed mitochondrial structure in C. elegans fed either E. coli OP50 or E. coli HT115. Under normal conditions, mitochondrial quality control involves constant fission and fusion events that serve to pool healthy, functional mitochondrial content, while damaged material is sequestered for autophagic recycling . A C. elegans strain expressing a mitochondrially-targeted GFP  was reared on E. coli OP50 or E. coli HT115 with or without methylcobalamin supplementation, and mitochondria were imaged in the same body wall muscle cell of young adult C. elegans. Worms fed E. coli HT115 or bacteria supplemented with methylcobalamin showed increased connectivity and fewer punctae than worms with less B12 (Fig 3A and 3B). The fragmentation induced by a diet of E. coli OP50 was greater than that observed when RNAi was used to knock down fzo-1/MFN, a mitofusin essential for proper mitochondrial fusion and homeostasis (S8 Fig).
(A) glp-4(bn2ts); zcIs14|myo-3::GFP(mt) worms, encoding a mitochondrially-targeted GFP were fed E. coli OP50 or E. coli HT115 with or without methylcobalamin supplementation. Body wall muscle mitochondria were imaged in the same tail cell of worms from each condition. Worms were grouped into high, medium, or low connectivity, as shown by inset images. (B) Quantification of mitochondrial phenotypes from (A). (C) Relative abundance of mitochondrial genome count in worms fed on E. coli OP50 or E. coli OP50 supplemented with methylcobalamin. (D) Measurement of mitochondrial membrane staining with nonyl-acridine orange (NAO). (E,F) Mitochondrial membrane potential, as determined by staining with MitoTracker Red (E) or tetramethylrhodamine ester (TMRE) (F), in worms fed as in (A). (G) Measurement of ROS production in worms, measured via fluorescence of dihydroethidium, fed as in (A). (H) ATP production in worms fed as in (A). Luminescence was normalized to GFP fluorescence to control for protein expression. *—p<0.05, p-value was calculated based on Student’s t-test. For (B) at least 30 worms were used per diet per biological replicate. For (C-G) at least 2,000 worms were used per biological replicate. For (H) at least 4 wells with 100 worms per well per condition per replicate. At least three biological replicates were performed for each experiment.
Breakdown of the mitochondrial network is commonly associated with reduced organellar function. We assayed other metrics of mitochondrial health in worms reared on E. coli OP50 or E. coli HT115 with or without exogenous vitamin B12. Methylcobalamin supplementation slightly, but statistically significantly, decreased the average mitochondrial genome count as measured by quantitative PCR of mitochondrial to nuclear genome count (Fig 3C). Mitochondrial mass was slightly diminished when measured using nonyl-acridine orange staining (NAO, Fig 3D). Two different dyes to measure mitochondrial membrane potential (tetramethylrhodamine ethyl ester (TMRE) and mitotracker red (MTR)) showed no significant difference on any of the diets (Fig 3E and 3F), which suggested that B12 may slightly improve the average mitochondrial membrane potential. Supplementation with methylcobalamin reduced superoxide production as an indicator of ROS in worms fed OP50, but did not have a significant effect on worms reared on HT115 (p = 0.059) (Fig 3G). ATP production (as measured by luciferase activity) showed no significant difference after B12 supplementation (Fig 3H). Combined, these data indicate that B12 sufficiency correlates with an increase in mitochondrial connectivity and decreased mitochondrial number. This permits mitochondrial function to be carried out at a similar level with fewer mitochondria.
Vitamin B12 supplementation increases stress resistance
We also tested whether methylcobalamin supplementation could alleviate the broad-spectrum sensitivity exhibited by E. coli OP50-fed worms. Worms were reared on E. coli OP50 grown with or without exogenous methylcobalamin, and their survival was tested in Liquid Killing. A dramatic difference was observed; less than half of OP50-fed worms remained alive by the time ~10% of OP50/B12-fed worms died (Fig 4A and 4B). Increased vitamin B12 availability also improved resistance to phenanthroline, infection with E. faecalis, peroxide stress, the mitochondrial poison carbonyl cyanide m-chlorophenyl hydrazone (CCCP), and hyperthermia (Fig 4C–4G). The resistance of wild-type worms fed on E. coli OP50 supplemented with methylcobalamin was also increased (S9 Fig).
(A-B) Representative images and quantification of survival of glp-4 (bn2) C. elegans exposed to P. aeruginosa PA14 after feeding on OP50 with or without methylcobalamin (B12) supplementation. (C-F) Effect of feeding on E. coli OP50 supplemented with methylcobalamin on C. elegans resistance to phenanthroline (C), infection with E. faecalis (D), peroxide exposure (E), CCCP poisoning (F), or hyperthermia (G), or lifespan (F). p-value for (E) <0.01; (F) > 0.05 (N.S). p-values were calculated using log-rank test (E, F) or Student’s t-test (B-D). *—p<0.01. For (A, B, D, E, F), 10 wells, each containing 20 worms, were used for each diet for each replicate. For (C, G, H), 50 worms were used per plate, three plates per replicate per condition. Three biological replicates were performed for each experiment.
A growing body of evidence suggests that decreasing mitochondrial activity, either by genetically compromising oxidative phosphorylation or by caloric restriction, extends lifespan [63,64]. Lifespan was unaffected by methylcobalamin supplementation (Fig 4H), as was seen when E. coli OP50 was replaced with E. coli HT115 (Fig 1G).
The E. coli TonB transporter mediates bacterial vitamin B12 uptake
All of these observations suggest that E. coli OP50 provides inadequate vitamin B12 for C. elegans. Since E. coli cannot synthesize vitamin B12, the bacterium must import it from the extracellular milieu, a process that has been reported to require TonB [65,66]. On this basis, we hypothesized that a bacterial strain lacking tonB would also trigger B12 deficiency in C. elegans. This prediction was tested with two different tonB deletions in E. coli BW25113 . To establish a baseline, expression of acdh-1p::GFP was determined for C. elegans reared on E. coli BW25113. This diet largely recapitulated acdh-1p::GFP levels observed for E. coli OP50 (Fig 5A), indicating that this diet also likely causes a vitamin B12 deficiency. As with E. coli OP50 and E. coli HT115, supplementation of wild-type BW25113 with methylcobalamin completely abolished acdh-1p::GFP fluorescence (Fig 5B). qRT-PCR data on log phase growth cultures of each strain indicate that tonB levels for E. coli HT115 are approximately 12 times higher than E. coli OP50 or E. coli BW25113 (Fig 5C). Although tonB is important for the import of several large molecules, such as cobalamin, nickel complexes, and some carbohydrates , it is also required for infection by several bacteriophages , suggesting that there may be an evolutionary advantage in limiting its expression.
(A) Box plot representation of basal acdh-1∷GFP expression in E. coli OP50, E. coli HT115, or E. coli BW25113. (B) Flow vermimetry measurements of the acdh-1p::GFP reporter fed with E. coli BW25113 with or without methylcobalamin (200 ng/mL) supplementation. (C) Relative level of tonB mRNA in panel of E. coli as in (A). (D) Flow vermimetry measurements of the acdh-1p::GFP reporter fed with an E. coli OP50, OP50 + pBAD, or OP50 + pBAD-OPtonB (tonB overexpression). *—p<0.01 based on Student’s t-test. For (A, B, D), at least 2,000 worms were used per condition per biological replicate. Three biological replicates were performed for each experiment.
To determine whether this limitation in tonB expression could be overcome, the tonB locus was cloned into pBAD for inducible expression and the resulting construct was transformed into E. coli OP50. tonB expression was induced with 0.2% L-arabinose in LB media unsupplemented with methylcobalamin and then bacteria were spotted onto NGM. Worms were reared on this food source, and acdh-1p::GFP expression was assayed in young adults. A small, but statistically significant and repeatable reduction in acdh-1p::GFP fluorescence was seen (Fig 5D). It is unclear why the overexpression did not have a more pronounced effect. One possibility is that overexpression of TonB, which is present in the cytoplasmic membrane , prevents it from being properly folded and/or inserted into the membrane. Additionally, TonB is a member of a protein complex; altering the stoichiometry of proteins in complexes by overexpression often results in unpredictable consequences and poor expression, which has led to the 'balance hypothesis' [71–73]. Either, or both, of these phenomena may have limited the proper expression or function of TonB.
Surprisingly, neither tonB deletion allele completely blocked the attenuation of acdh-1p::GFP fluorescence seen from methylcobalamin supplementation (S10 Fig). This suggests that the bacteria may have an alternative, tonB-independent route to obtain cobalamin, although the process appears to be inefficient. Alternatively, the cells may be generating B12 de novo by salvaging precursors that they can convert into B12.
B12-dependent resistance relies upon the methylmalonate-CoA/succinyl-CoA pathway of propionate breakdown
There are three obvious explanations for the vitamin B12-mediated resistance we observed. First, the additional vitamin B12 may alter the metabolism of E. coli (e.g., a deficiency of vitamin B12 in the LB broth used may limit the quality of the nutrition provided by the E coli, supplementation decreases the production of a toxic bacterial metabolite, or the bacteria may increase production of one or more salubrious compounds). Second, the bacterium may modify or metabolize the vitamin, creating the product that improves health. Finally, the bacteria may merely be the means of transporting the B12 into the intestine of C. elegans, where it directly alters host metabolism. To rule out the first two possibilities, we spotted heat-killed E. coli onto NGM plates that were themselves supplemented with methylcobalamin. glp-4(bn2) worms spotted onto these plates also exhibited increased resistance to P. aeruginosa Liquid Killing (S11 Fig).
On this basis, it was clear that E. coli is merely a vehicle for transporting vitamin B12 into C. elegans. As noted above, vitamin B12 functions as an essential co-factor for two enzymes: METR-1/MTR and MMCM-1/MUT (Fig 6A) . To determine which of these functions underlies the improvement conferred by vitamin B12, survival in Liquid Killing was assessed in worms with mutations for each pathway.
(A) Schematics of biochemical pathways for methionine and propionyl-CoA metabolism in C. elegans. Proteins in red utilize B12 as a cofactor. (B) Survival of C. elegans fed on E. coli HT115 carrying empty vector or metr-1(RNAi) with or without exogenous methylcobalamin after exposure to P. aeruginosa PA14. (C) Survival of C. elegans reared on E. coli OP50 or OP50 supplemented with L-methionine after P. aeruginosa PA14 exposure. (D-F) Survival of wild-type C. elegans or mutants in two different propionate breakdown pathways with or without methylcobalamin supplementation after P. aeruginosa PA14 exposure. NS–p>0.05, *—p<0.01 based on Student’s t-test. For (B, C, D, E, F) 10 wells, each containing 20 worms, are used per condition per replicate. Three biological replicates were performed for each experiment.
RNAi targeting either metr-1/MTR or mtrr-1/MTRR had no effect on vitamin B12-mediated resistance to P. aeruginosa in the Liquid Killing assay (Fig 6B). To rule out the possibility of incomplete or insufficient RNAi knockdown, we also tested whether supplementing bacteria with 3 mM methionine (instead of methylcobalamin) improved host survival. Since this pathway uses vitamin B12 to generate methionine, supplementation with this amino acid should have the same result if this pathway is relevant. Consistent with the results from the metr-1(RNAi) and mtrr-1(RNAi) mutants, methionine supplementation had no impact on survival (Fig 6C). In contrast, disruption of the other B12-utilizing pathway abolished resistance even in the presence of exogenous methylcobalamin. RNAi targeting mce-1/MCEE or mutation of mmcm-1/MUT completely abolished the benefit from methylcobalamin supplementation (Fig 6D and 6E).
C. elegans maintains an alternative, B12-independent, pathway to metabolize propionyl-CoA. This shunt is more toxic and utilizes acrylyl-CoA and hydroxypropionyl-CoA intermediates . We also tested whether this pathway plays a role in mitochondrial toxicity of dietary B12 deficiency. Mutations in hphd-1/ADHFE1 or alh-8/ALDH6A1, two genes in this shunt, had no effect on the ability of vitamin B12 supplementation to promote survival (Fig 6F). This further supports our conclusion that the MMCM-1/MUT pathway is the relevant target for B12-mediated improvements in host health.
While probing the mechanisms of pathogenesis of P. aeruginosa in C. elegans, we discovered that switching between two commonly used strains of E. coli, OP50 and HT115, dramatically altered host stress tolerance. Further investigation linked these differences to improved mitochondrial homeostasis in worms reared on E. coli HT115 and suggest that this is likely due to the buildup of propionyl-CoA, a mitotoxic byproduct of branched chain amino acid metabolism, in worms reared on E. coli OP50.
Normally, propionyl-CoA is converted to succinyl-CoA, via a methylmalonyl-CoA intermediate, in a vitamin B12-dependent fashion. However, several lines of evidence, as well as previous reports, suggest that a diet of E. coli OP50 generates a vitamin B12 deficiency in the host. It is worth noting that this deficiency is likely to be relatively mild, since severe vitamin B12 deficiency causes drastic phenotypes in C. elegans, including infertility, growth retardation, and shortened lifespan . However, we saw no gross differences in growth rate or lifespan in worms when they were provided with E. coli HT115 or E. coli OP50 supplemented with methylcobalamin as compared to E. coli OP50 alone.
Several lines of evidence support our conclusion that E. coli HT115 is a better source of vitamin B12 than E. coli OP50. For example, worms reared on E. coli HT115 had diminished acdh-1p::GFP fluorescence and decreased propionate toxicity. Moreover, supplementation of an OP50 diet with methylcobalamin conferred HT115-like characteristics in terms of mitochondrial homeostasis and vitamin B12 phenotypes. Tellingly, RNAi targeting mce-1/MCEE or mmcm-1/MUT mutations abolished the health improvement conferred by methylcobalamin supplementation, indicating that this pathway and this metabolite were involved. Moreover, worms reared on E. coli OP50 grown in minimal media showed delays in egg-laying compared to worms fed E. coli OP50 supplemented with vitamin B12 or E. coli HT115 (S12 Fig). Worms serially passaged on foods grown in this media also showed a substantial reduction in fecundity after 5 generations. Both of these findings are consistent with previous reports [20,23] and are indicative of acute and chronic vitamin B12 deficiency. Finally, elegant work by the Walhout group has indicated a vitamin B12 deficiency in OP50-reared worms .
Increased pathogen sensitivity from B12 deficiency may be evolutionarily conserved
While malnutrition is well-known to predispose animals to infection, subtle nutritional defects, and their concomitant effects on host physiology, are more difficult to detect. Interestingly, our findings may explain an intriguing finding from a recently published study . Gif mutant mice, which have compromised intestinal absorption of dietary B12, showed a striking increase in sensitivity and mortality to infection with Salmonella enterica serovar Typhimurium or Citrobacter rodentium. Although the infected mice showed no overt immune deficiencies, they had severe metabolic defects that included compromised mitochondrial function and dramatic increases in methylmalonate concentration. Importantly, these phenotypes were resolved by supplementation of the animals' diet with cobalamin. The authors postulated that the increased mortality may arise from metabolic starvation due to competition for nutrients between the host and its microbiota. However, their results can also be explained by our model. I.e., the mitochondrial damage inflicted by vitamin B12-deficiency made the host more sensitive to stress and pathogens and significantly increased mortality. Although published analyses are limited, there is also some evidence to suggest people with genetic priopionate acidemias, which similarly cause propionyl-CoA accumulation, may also be predisposed to bacterial and fungal infections .
A consistent, defined diet is needed for C. elegans
Although we began our queries of the host-microbiota-diet axis with a minimal, binary system (C. elegans and E. coli), unexpected complexity has arisen. Differences in the biology of C. elegans reared on OP50 or HT115 have generally been attributed to the differences in the origins of the bacterial strains (i.e., OP50 was derived from an E. coli B strain while HT115 came from E. coli K12) or to their differences in nutrient composition (HT115 contains less triacylglycerols and pyrimidines, and more carbohydrates than OP50 [8,77] and increases host concentrations of some amino acids and other metabolites ). Our data suggest that acdh-1p::GFP expression, a marker for B12 deficiency, poorly correlates with strain origin. E. coli BW25113, which also originated from K12, showed acdh-1p::GFP fluorescence similar to OP50 (Fig 5A)).
Metabolic differences of this sort likely contribute substantial uncertainty to research outcomes, particularly since some labs use E. coli OP50 as the standard food, some use E. coli HT115, and others routinely use E. coli HB101. For example, despite the fact that the C. elegans literature is replete with comparisons of the lifespan of C. elegans reared on OP50 vs. HT115, no consensus conclusion has been reached. Some researchers have seen no difference in lifespan [8,45], others find an HT115-mediated extension of lifespan [9,78], and still others find OP50-reared worms surviving longer . Explanations for these divergences abound, including variations in media composition (or even batch-to-batch variations from a single supplier), methodological differences in assays, or even accumulated mutations in the "wild-type" E. coli or C. elegans strains as they are propagated within and between labs.
Ultimately, the inability to resolve what should be a simple question (i.e., which food allows C. elegans to live longer?) is troubling, particularly since the phenotype being assayed (i.e., death) should be unambiguous and the experimental setup is straightforward. More elusive phenotypes with perhaps smaller effects and more complex experimental design likely have greater variability. Curran and colleagues  have persuasively argued the need for a rigorously-defined, standardized growth medium for studies of aging in C. elegans; our data suggest this need probably extends to all studies using this model.
Materials and methods
C. elegans strains
All C. elegans strains were maintained on nematode growth medium (NGM) seeded with Escherichia coli strain OP50, E. coli strain HT115, or E. coli BW25113 (see below). In some experiments, E. coli growth media were supplemented with methylcobalamin to a final concentration of 0.2 mg/L. Unless otherwise noted, worms were reared and passaged at 15°C , with the exception of glp-4(bn2) worms, which were sterilized prior to use by plating diapaused, synchronized L1 larvae on concentrated E. coli on NGM plates and kept at 25°C. For RNAi-mediated gene knockdown, plasmids from the Ahringer library  were either used in the E. coli HT115(DE3) strain supplied or were purified and transformed into E. coli OP50(xu363), an RNAi-competent strain of OP50 . All plasmids were sequence verified.
C. elegans strains used in this study included N2 Bristol (wild-type), SS104 [glp-4(bn2ts)] , NVK44 [glp-4(bn2ts); zcIs14|myo-3::GFP(mt)|], PE327 (ATP reporter): glp-4(bn2ts); feIs5 [sur-5p::luciferase::GFP + rol-6(su1006)] , RB1434[mmcm-1(ok1637)], RB2572[hphd-1(ok3580)], VL1176[alh-8(ww48)], and VL749 [wwIs24|acdh-1p::GFP + unc-119(+)|] .
Bacterial strains used in this study included E. coli OP50, E. coli OP50(xu363) , E. coli HT115(DE3), and E. coli BW25113. Two E. coli tonB deletion alleles (JW5195-1 and JW5195-2) were taken from the Keio Knockout Collection (GE Dharmacon). To generate the tonB overexpression strain, genomic DNA was purified from E. coli strain OP50 used to amplify the tonB locus. The resultant PCR product was digested with NdeI and SalI and subcloned into pBAD33.1 (a gift from Christian Raetz, Addgene plasmid #36267 ). The resultant plasmid, pBAD-OPtonB was transformed into chemically competent E. coli OP50 using conventional techniques. For pathogenesis assays, P. aeruginosa strain PA14 , P. aeruginosa PA14 tranformed to express DsRed , or E. faecalis strain OG1RF  were used.
Heat-Killed E. coli OP50
To prepare heat-killed E. coli OP50, E. coli from an overnight culture in LB were centrifuged and concentrated tenfold in S Basal. Bacteria were then killed by incubation at 75°C for 30 min with regular mixing by inversion. Absence of live E. coli in each preparation was confirmed by plating on LB agar.
For use in Liquid Killing assays, 2 mL of concentrated dead bacteria were plated onto modified NGM that was supplemented with vitamin B2 to a final concentration of 0.3 mg/L. Normally, C. elegans grows poorly on dead E. coli. However, exogenous vitamin B2 significantly improves C. elegans health under these conditions . To test vitamin B12 supplementation, the NGM also supplemented with 0.2 mg/L methylcobalamin.
C. elegans pathogenesis, chemical exposure, hyperthermia, and longevity assays
Liquid Killing assays with P. aeruginosa PA14 were performed as described . The C. elegans—E. faecalis assay was performed as described . Assays were timed such that ~60–70% worms reared on E. coli OP50 would be dead. At least three biological replicates were performed per condition per experiment. Each biological replicate contained at least 10 wells (~200 animals). Statistical significance was determined using Student’s t-test.
For the juglone survival assay, glp-4(bn2) worms were grown to young adulthood and placed on NGM agar media supplemented with 120 μM of juglone . For peroxide and carbonyl cyanide m-chlorophenyl hydrazone (CCCP) exposure worms were treated with 2 mM or 100 μM of drug in S Basal, respectively. Survival was scored using Sytox Orange stain after 20 h of incubation. Phenanthroline survival assays were done similarly, except plates were supplemented with 100 μM of this chelator. In each case, plates were made fresh and used the same day. Hyperthermia assays were performed at 30°C. In all cases, unsupplemented NGM agar plates incubated at 25°C were used as controls. Worms were scored daily and worms were scored as dead when they failed to respond to touch. Longevity assays were performed similarly, except worms were incubated at 25°C on the appropriate food source for the duration of the experiment and scored every other day. Worms were considered dead when they failed to respond to a gentle prod to the head. At least three biological replicates were performed for each experiment. Each biological replicate consisted of three plates with ~50 worms/plate. Statistical significance was determined using log-rank test (http://bioinf.wehi.edu.au/software/russell/logrank/). Worms on plates were censored if they left the agar plate.
The propionate sensitivity assay was performed as described in  with modifications. 70 L1-stage worms were dropped on to NGM agar plates containing appropriate concentrations of propionate (or no propionate control) using a COPAS FlowSort. After 72 h incubation at 25°C, adult worms were counted and survival was calculated. At least three biological replicates were performed for each experiment. Statistical significance was determined using Student’s t-test.
Detection of total iron via ICP-MS
In brief, approximately 24,000 C. elegans L1 larvae (per sample) were raised on NGM plates seeded with E. coli OP50 or E. coli HT115. Upon reaching young adulthood, worms were transferred to 15 mL conicals, washed four times, and then collected with identical volumes. Samples were frozen at -80°C and processed as described . At least three replicates were tested for each diet. Significance was tested using Student's t-test.
Detection of host ferric iron
glp-4(bn2) L1 larvae were spotted onto NGM plates seeded with either E. coli OP50 or E. coli HT115 and allowed to develop to young adulthood at 25°C. Worms were collected, lysed, and fluorometric determination of ferric iron was performed as previously described .
For RNA collection, glp-4(bn2ts) worms were grown on appropriate plates until reaching young adult stage. Three biological replicates were performed. RNA was purified using Trizol following by cleanup according to Qiagen protocol. cDNA and cRNA were synthesized and hybridized to Affymetrix GeneChips for C. elegans at the Partners Center for Personalized Genetic Medicine, Boston, MA, according to manufacturer’s protocols. Three biological replicates were tested for each condition. Gene expression was analyzed using GCRMA (http://www.bioconductor.org). Differentially regulated genes were determined on the basis of fold change (>2) and the value of a modified Wilcoxon rank test (>1.5). The Wilcoxon coefficient was determined for each probeset as the smallest expression value in the condition with higher average divided by the highest expression value in the condition with lower average. Microarray data were deposited in GEO database and are available using following link: https://www.ncbi.nlm.nih.gov/geo/query/acc.cgi?token=kjibcyuydrstvuj&acc=GSE97678
Quantitative Real-Time PCR (qRT-PCR)
For determination of the basal level of immune genes in C. elegans, ~10,000 of OP50- and HT115-fed glp-4(bn2ts) worms were grown to young adult stage and RNA was purified as described above. cDNA synthesis was performed according to manufacturers’ protocols (Ambion). qRT-PCR was performed using SYBR Green iQ mix (Bio-Rad). snb-1 gene was used as a control. For each gene, threshold cycle (Ct) was determined and ΔCt from snb-1 was calculated.
For measurement of relative abundance of mitochondrial DNA, total DNA was extracted from ~2,000 synchronized young adult worms grown on appropriate food source. For genome comparisons, nd1 was used as a mitochondrial gene and act-3 as nuclear, as previously described . Resultant DNA was used for to perform quantitative PCR using SYBR Green (BioRad), and mitochondrial gene level was normalized to nuclear gene number using the ΔΔCt method. Thermocycler parameters were as for qRT-PCR.
For measurements of tonB expression in E. coli strains, RNA was purified as described above, except samples were treated with DNAase I (NEB). cysG and idnT were used as housekeeping genes . Fold changes were calculated using ΔΔCt method.
Primer sequences are available upon request. Three biological replicates were performed per test, each biological replicate contained duplicate wells for each primer/cDNA combination. Statistical significance was calculated using Student’s t-test.
For visualization of myo-3::GFP(mt) and acdh-1p::GFP on slides, L1 larvae were spotted onto NGM plates seeded with appropriate bacteria, and allowed to mature into young adults at 25°C. Worms were immobilized with levamisole and transferred to slides. Images were acquired using a Zeiss Axio Imager M2 upright microscope with a Zeiss AxioCam 506 Mono camera and Zeiss Zen2Pro software. All fluorescent images were collected under identical exposure conditions. Fluorescence quantification was based on at least 50 worms per condition per biological replicate. At least three biological replicates were performed. Statistical significance was determined by Student’s t-test.
ATP determination in live worms
For determination of ATP concentrations, approximately 2,000 PE327 L1 larvae  were placed onto NGM plates seeded with either E. coli OP50 or E. coli HT115 and allowed to develop to young adult stage at 25°C. Worms were then transferred to 96-well, white clear bottom plates and washed with S-basal five times. 150 μL Luminescence buffer (0.14M K2PO4, 0.03M sodium citrate, 1% DMSO, 1mM luciferin) was added to each well in the plate. Bioluminescence and GFP fluorescence were measured after 30 min using a Cytation5 multimode plate reader/imager (BioTek). Luminescence values were normalized to GFP fluorescence to control for differences in protein expression.
For measurement of acdh-1p::GFP, 5,000 VL749 L1 larvae were spotted onto NGM plates seeded with the food sources described. In some cases, NGM was supplemented with propionate and/or methylcobalamin. Worms were collected into 50 mL conicals, washed three times, and then GFP fluorescence was measured using a COPAS FlowPilot with 488 nm excitation and a long-pass filter.
Mitochondrial membrane potential and reactive oxygen species were measured in a similar fashion, except that glp-4(bn2) worms were used, and worms were stained as described for MitoTracker Red . nonyl-acridine orange (NAO) and tetramethylrhodamine ester (TMRE) dyes were used to stain mitochondria at 10 μM and 5 μM, respectively. ROS measurements were performed similarly, except dihydroethydium at a concentration of 3 μM and excitation at 488 nm was used. In each case, worms were stained for 1h, then washed 5 times prior to being measured. Measurements for each stain/diet combination were taken with the same settings. At least 1,500 worms/condition/biological replicate were used; at least three biological replicates were performed. Statistical significance was determined by Student’s t-test.
Worm fecundity was scored as described by Bito et al.,  with minor modifications. E. coli OP50, HT115, and OP50 supplemented with 100 μM methylcobalamin were grown for 3 days in M9 medium at 37°C, then concentrated and plated onto normal NGM. Single glp-4(bn2) larvae were transferred to a new plate containing the same food. After reaching late-L4 stage, worms were allowed to lay eggs for 24 h. Young adult worms were then transferred to a fresh plate with the same food and allowed to complete egg laying. After 48 h, progeny on both plates were counted (providing both the 24h count and the total count). One larva, chosen arbitrarily, was transferred to a new plate, to yield progeny for the subsequent generation. At least 24 plates were used per strain per biological replicates per generation; three biological replicates were performed. Statistical significance was determined by Student’s t-test.
S1 Fig. E. coli OP50 and E. coli HT115-fed C. elegans have similar iron content.
(A) The presence of the empty pL4440 vector did not affect survival in Liquid Killing. (B) Relative abundance of ferric iron in worms fed E. coli OP50 or E. coli HT115. (C) ICP-MS analysis of total iron concentration in worms fed E. coli OP50 or E. coli HT115. N.S.—p > 0.05. based on Student’s t-test. For (A) 10 wells, each containing 20 worms, were used per condition per replicate. For (B), approximately 18,000 worms were used per biological replicate per condition. For (C), approximately 24,000 worms were used per biological replicate per condition. Three biological replicates were performed for each experiment.
S2 Fig. E. coli HT115 does not affect P. aeruginosa slow killing.
(A) glp-4(bn2) worms were reared on E. coli OP50 or E. coli HT115 and then used for P. aeruginosa PA14 slow-killing. (B-C) Fluorescent images (B) or quantification of fluorescence (C) of colonization by P. aeruginosa PA14-DsRed during slow kill assays after being reared on OP50 or HT115. Statistical significance was calculated based on log-rank test (A) or Student’s t-test (C). No significant changes were observed. For (A), 50 worms per plate, three plates per condition per replicate were used. For (B), 30 worms per plate, three plates per condition per replicate were used. Three biological replicates were performed for each experiment.
S3 Fig. A diet of E. coli HT115 does not change basal levels of expression of innate immune or stress pathway effector genes.
(A-E) qRT-PCR analysis of gene expression levels for downstream effectors from the indicated innate immune or stress response pathway. p>0.05 for all primers tested. Statistical significance was calculated based on Student’s t-test. No significant changes were observed. About 10,000 worms were used per biological replicate per condition. Three biological replicates were performed for each experiment.
S4 Fig. Worms fed E. coli OP50(xu363) and E. coli HT115 have similar sensitivity to RNAi.
Starting at the L4 stage, C. elegans were fed RNAi-competent strains of E. coli OP50(xu363) or E. coli HT115 bacteria that contained plasmids driving expression of cyc-1 RNAi constructs (which results in embryonic lethality). Each worm was placed onto an individual plate and moved to fresh plate daily. NS–p>0.05 based on Student’s t-test. At least 30 adults were used per biological replicate per condition. Three biological replicates were performed.
S5 Fig. E. coli HT115-mediated resistance is not dependent upon activation of canonical innate immune or stress response pathways.
(A-E) Starting at the L1 stage, C. elegans were fed E. coli OP50 or E. coli HT115 bacteria that contained plasmids driving expression of RNAi constructs that targeted innate immune or stress response genes. Young adult worms were subsequently exposed to P. aeruginosa PA14 for an appropriate length of time. Percent survival was inferred based on staining with Sytox Orange, a cell impermeant dye. *—p<0.01 based on Student’s t-test. 10 wells, 20 worms per well, were used per condition per biological replicate. Three biological replicates were performed for each experiment.
S6 Fig. Methylcobalamin supplementation improves survival of wild-type worms.
(A-C) Survival of wild-type (N2) C. elegans worms fed E. coli OP50 alone or supplemented with methylcobalamin or E. coli HT115-fed worms in P. aeruginosa-mediated Liquid Killing (A), propionate intoxication (B), or hyperthermia at 30°C (C). (D) Longevity of worms reared as in (A). *—p< 0.01, based on Student’s t-test. For (C, D) p<0.01 was calculated using a log-rank test. For (A), ten wells, with 20 worms per well, were used for each condition for each replicate. For (B-D), 70 (B) or 50 (C, D) worms per plate, three plates per condition were used per replicate. Three biological replicates were performed for each of the experiments.
S7 Fig. Quantification of acdh-1p::GFP expression.
(A) Quantification of acdh-1p::GFP reporter fluorescence in worms fed either E. coli OP50 or E. coli HT115, with or without methylcobalamin supplementation to a final concentration of 200 ng/ml, as indicated. (B) Quantification of acdh-1p::GFP expression in worms fed E. coli OP50 or E. coli HT115, with or without methylcobalamin supplementation to a final concentration of 200 ng/ml and exposed to propionate, using flow vermimetry. Fluorescence for each worm was normalized to its size. *—p<0.01 based on Student’s t-test. For (A) 30 worms per condition per replicate were measured. For (B), 2,000 worms were used per biological replicate per condition, a representative replicate is shown. Three biological replicates were performed for each experiment.
S8 Fig. Fzo-1/Mfn1(RNAi) induces mitochondrial fragmentation.
glp-4(bn2ts); myo-3::GFP(mt) worms were reared on either E. coli HT115 containing either an empty RNAi vector or an RNAi vector targeting fzo-1/Mfn1 and then imaged to evaluate fragmentation of the mitochondrial network. Fragmentation was assessed as in Fig 3. 30 worms were used for each condition for each replicate. Three biological replicates were performed for each experiment.
S9 Fig. Methylcobalamin supplementation improves resistance to mitochondrial poisons in wild-type worms.
Wild-type (N2) worms were reared on E. coli OP50 with or without methylcobalamin supplementation and then exposed to toxic levels of either peroxide (A) or CCCP (B). 10 wells, with 20 worms per well, were used for each condition for each replicate. At least 2 biological replicates were performed for each experiment. *—p<0.01 based on Student’s t-test.
S10 Fig. E. coli BW25113 has a tonB-independent method for vitamin B12 import.
achd-1p::GFP was measured via flow vermimetry in worms reared on two different tonB deletion strains in the E. coli BW25113 background sourced from the Keio collection. Bacteria were grown with and without exogenous methylcobalamin.
S11 Fig. Methylcobalamin supplementation improves survival independently of bacteria.
Survival of C. elegans reared on heat-killed E. coli OP50. NGM agar was either supplemented or not with 200 ng/mL of methylcobalamin. Worms were exposed to P. aeruginosa PA14 and survival was assessed after 42 h.
S12 Fig. Bacterial media deficiency causes long-term changes to C. elegans fecundity.
24h and total brood sizes were determined for wild-type (N2) worms reared on E. coli OP50 with or without exogenous methylcobalamin, or E. coli HT115 that was grown in minimal M9 media. L4 larvae were transferred to fresh plates with the same food, allowed to lay for 24h and then were transferred to a new plate for another 24h. Fecundity was assessed by counting the number of hatched larvae. For each condition, 30 worms were tested per replicate per generation; at least three biological replicates were performed.
S1 Table. List of genes differentially regulated by feeding on E. coli HT115 vs. E. coli OP50.
Genes differentially regulated in young adult glp-4(bn2) worms, grown on E. coli HT115 since L1 stage. Fold changes shown are normalized to the genes’ expression levels in E. coli OP50.
S2 Table. Common genes between two transcriptome profiling studies on the effect of HT115 on C. elegans transcriptome.
Microarray data on genes that were up- or down-regulated when worms were fed E. coli HT115 (as compared to the standard laboratory diet of E. coli OP50) were compared between  and this study.
We wish to thank Alex Kang and Dr. Chris Pennington for technical assistance with ICP-MS. E. coli OP50(xu363) was provided by Dr. Eyleen O’Rourke, E. faecalis OG1RF was the kind gift of Dr. Danielle Garsin. Some strains were provided by the CGC, which is funded by NIH Office of Research Infrastructure Programs (P40 OD010440).
- 1. Leulier F, MacNeil LT, Lee WJ, Rawls JF, Cani PD, et al. (2017) Integrative Physiology: At the Crossroads of Nutrition, Microbiota, Animal Physiology, and Human Health. Cell Metab 25: 522–534. pmid:28273475
- 2. Org E, Parks BW, Joo JW, Emert B, Schwartzman W, et al. (2015) Genetic and environmental control of host-gut microbiota interactions. Genome Res 25: 1558–1569. pmid:26260972
- 3. Ussar S, Griffin NW, Bezy O, Fujisaka S, Vienberg S, et al. (2015) Interactions between Gut Microbiota, Host Genetics and Diet Modulate the Predisposition to Obesity and Metabolic Syndrome. Cell Metab 22: 516–530. pmid:26299453
- 4. Rothschild D, Weissbrod O, Barkan E, Kurilshikov A, Korem T, et al. (2018) Environment dominates over host genetics in shaping human gut microbiota. Nature 555: 210–215. pmid:29489753
- 5. Cabreiro F, Gems D (2013) Worms need microbes too: microbiota, health and aging in Caenorhabditis elegans. EMBO Mol Med 5: 1300–1310. pmid:23913848
- 6. MacNeil LT, Watson E, Arda HE, Zhu LJ, Walhout AJ (2013) Diet-induced developmental acceleration independent of TOR and insulin in C. elegans. Cell 153: 240–252. pmid:23540701
- 7. Reinke SN, Hu X, Sykes BD, Lemire BD (2010) Caenorhabditis elegans diet significantly affects metabolic profile, mitochondrial DNA levels, lifespan and brood size. Mol Genet Metab 100: 274–282. pmid:20400348
- 8. Brooks KK, Liang B, Watts JL (2009) The influence of bacterial diet on fat storage in C. elegans. PLoS One 4: e7545. pmid:19844570
- 9. Maier W, Adilov B, Regenass M, Alcedo J (2010) A neuromedin U receptor acts with the sensory system to modulate food type-dependent effects on C. elegans lifespan. PLoS Biol 8: e1000376. pmid:20520844
- 10. Saiki R, Lunceford AL, Bixler T, Dang P, Lee W, et al. (2008) Altered bacterial metabolism, not coenzyme Q content, is responsible for the lifespan extension in Caenorhabditis elegans fed an Escherichia coli diet lacking coenzyme Q. Aging Cell 7: 291–304. pmid:18267002
- 11. Lenaerts I, Walker GA, Van Hoorebeke L, Gems D, Vanfleteren JR (2008) Dietary restriction of Caenorhabditis elegans by axenic culture reflects nutritional requirement for constituents provided by metabolically active microbes. J Gerontol A Biol Sci Med Sci 63: 242–252. pmid:18375873
- 12. Garsin DA, Villanueva JM, Begun J, Kim DH, Sifri CD, et al. (2003) Long-lived C. elegans daf-2 mutants are resistant to bacterial pathogens. Science 300: 1921. pmid:12817143
- 13. Gusarov I, Gautier L, Smolentseva O, Shamovsky I, Eremina S, et al. (2013) Bacterial nitric oxide extends the lifespan of C. elegans. Cell 152: 818–830. pmid:23415229
- 14. Virk B, Correia G, Dixon DP, Feyst I, Jia J, et al. (2012) Excessive folate synthesis limits lifespan in the C. elegans: E. coli aging model. BMC Biol 10: 67. pmid:22849329
- 15. Virk B, Jia J, Maynard CA, Raimundo A, Lefebvre J, et al. (2016) Folate Acts in E. coli to Accelerate C. elegans Aging Independently of Bacterial Biosynthesis. Cell Rep 14: 1611–1620. pmid:26876180
- 16. Cabreiro F, Au C, Leung KY, Vergara-Irigaray N, Cocheme HM, et al. (2013) Metformin retards aging in C. elegans by altering microbial folate and methionine metabolism. Cell 153: 228–239. pmid:23540700
- 17. Ding W, Smulan LJ, Hou NS, Taubert S, Watts JL, et al. (2015) s-Adenosylmethionine Levels Govern Innate Immunity through Distinct Methylation-Dependent Pathways. Cell Metab 22: 633–645. pmid:26321661
- 18. Krahenbuhl S, Chang M, Brass EP, Hoppel CL (1991) Decreased activities of ubiquinol:ferricytochrome c oxidoreductase (complex III) and ferrocytochrome c:oxygen oxidoreductase (complex IV) in liver mitochondria from rats with hydroxycobalamin[c-lactam]-induced methylmalonic aciduria. J Biol Chem 266: 20998–21003. pmid:1657942
- 19. Chandler RJ, Zerfas PM, Shanske S, Sloan J, Hoffmann V, et al. (2009) Mitochondrial dysfunction in mut methylmalonic acidemia. FASEB J 23: 1252–1261. pmid:19088183
- 20. Bito T, Matsunaga Y, Yabuta Y, Kawano T, Watanabe F (2013) Vitamin B12 deficiency in Caenorhabditis elegans results in loss of fertility, extended life cycle, and reduced lifespan. FEBS Open Bio 3: 112–117. pmid:23772381
- 21. Watson E, Yilmaz LS, Walhout AJ (2015) Understanding Metabolic Regulation at a Systems Level: Metabolite Sensing, Mathematical Predictions, and Model Organisms. Annu Rev Genet 49: 553–575. pmid:26631516
- 22. Watson E, MacNeil LT, Ritter AD, Yilmaz LS, Rosebrock AP, et al. (2014) Interspecies systems biology uncovers metabolites affecting C. elegans gene expression and life history traits. Cell 156: 759–770. pmid:24529378
- 23. Watson E, Olin-Sandoval V, Hoy MJ, Li CH, Louisse T, et al. (2016) Metabolic network rewiring of propionate flux compensates vitamin B12 deficiency in C. elegans. Elife 5.
- 24. Kirienko NV, Kirienko DR, Larkins-Ford J, Wählby C, Ruvkun G, et al. (2013) Pseudomonas aeruginosa disrupts Caenorhabditis elegans iron homeostasis, causing a hypoxic response and death. Cell Host Microbe 13: 406–416. pmid:23601103
- 25. Conery AL, Larkins-Ford J, Ausubel FM, Kirienko NV (2014) High-throughput screening for novel anti-infectives using a C. elegans pathogenesis model. Curr Protoc Chem Biol 6: 25–37. pmid:24652621
- 26. Kamath RS, Fraser AG, Dong Y, Poulin G, Durbin R, et al. (2003) Systematic functional analysis of the Caenorhabditis elegans genome using RNAi. Nature 421: 231–237. pmid:12529635
- 27. Rual JF, Ceron J, Koreth J, Hao T, Nicot AS, et al. (2004) Toward improving Caenorhabditis elegans phenome mapping with an ORFeome-based RNAi library. Genome Res 14: 2162–2168. pmid:15489339
- 28. Kirienko NV, Ausubel FM, Ruvkun G (2015) Mitophagy confers resistance to siderophore-mediated killing by Pseudomonas aeruginosa. Proc Natl Acad Sci U S A 112: 1821–1826. pmid:25624506
- 29. Kang D, Kirienko DR, Webster P, Fisher AL, Kirienko NV (2018) Pyoverdine, a siderophore from Pseudomonas aeruginosa, translocates into C. elegans, removes iron, and activates a distinct host response. Virulence 9: 804–817. pmid:29532717
- 30. Tjahjono E, Kirienko NV (2017) A conserved mitochondrial surveillance pathway is required for defense against Pseudomonas aeruginosa. PLoS Genet 13: e1006876. pmid:28662060
- 31. Anderson QL, Revtovich AV, Kirienko NV (2018) A High-throughput, High-content, Liquid-based C. elegans Pathosystem. J Vis Exp.
- 32. Yuen GJ, Ausubel FM (2014) Enterococcus infection biology: lessons from invertebrate host models. J Microbiol 52: 200–210. pmid:24585051
- 33. Win MT, Yamamoto Y, Munesue S, Han D, Harada S, et al. (2013) Validated Liquid Culture Monitoring System for Lifespan Extension of Caenorhabditis elegans through Genetic and Dietary Manipulations. Aging Dis 4: 178–185. pmid:23936742
- 34. Kim DH (2013) Bacteria and the aging and longevity of Caenorhabditis elegans. Annu Rev Genet 47: 233–246. pmid:24274752
- 35. Gomez F, Monsalve GC, Tse V, Saiki R, Weng E, et al. (2012) Delayed accumulation of intestinal coliform bacteria enhances life span and stress resistance in Caenorhabditis elegans fed respiratory deficient E. coli. BMC Microbiol 12: 300. pmid:23256533
- 36. Yu L, Yan X, Ye C, Zhao H, Chen X, et al. (2015) Bacterial Respiration and Growth Rates Affect the Feeding Preferences, Brood Size and Lifespan of Caenorhabditis elegans. PLoS One 10: e0134401. pmid:26222828
- 37. Dagda RK, Chu CT (2009) Mitochondrial quality control: insights on how Parkinson's disease related genes PINK1, parkin, and Omi/HtrA2 interact to maintain mitochondrial homeostasis. J Bioenerg Biomembr 41: 473–479. pmid:20012177
- 38. Dillin A, Hsu AL, Arantes-Oliveira N, Lehrer-Graiwer J, Hsin H, et al. (2002) Rates of behavior and aging specified by mitochondrial function during development. Science 298: 2398–2401. pmid:12471266
- 39. Papp D, Csermely P, Soti C (2012) A role for SKN-1/Nrf in pathogen resistance and immunosenescence in Caenorhabditis elegans. PLoS Pathog 8: e1002673. pmid:22577361
- 40. Estes KA, Dunbar TL, Powell JR, Ausubel FM, Troemel ER (2010) bZIP transcription factor zip-2 mediates an early response to Pseudomonas aeruginosa infection in Caenorhabditis elegans. Proc Natl Acad Sci U S A 107: 2153–2158. pmid:20133860
- 41. Kim DH, Liberati NT, Mizuno T, Inoue H, Hisamoto N, et al. (2004) Integration of Caenorhabditis elegans MAPK pathways mediating immunity and stress resistance by MEK-1 MAPK kinase and VHP-1 MAPK phosphatase. Proc Natl Acad Sci U S A 101: 10990–10994. pmid:15256594
- 42. Troemel ER, Chu SW, Reinke V, Lee SS, Ausubel FM, et al. (2006) p38 MAPK regulates expression of immune response genes and contributes to longevity in C. elegans. PLoS Genet 2: e183. pmid:17096597
- 43. Powell JR, Kim DH, Ausubel FM (2009) The G protein-coupled receptor FSHR-1 is required for the Caenorhabditis elegans innate immune response. Proc Natl Acad Sci U S A 106: 2782–2787. pmid:19196974
- 44. Timmons L, Court DL, Fire A (2001) Ingestion of bacterially expressed dsRNAs can produce specific and potent genetic interference in Caenorhabditis elegans. Gene 263: 103–112. pmid:11223248
- 45. Xiao R, Chun L, Ronan EA, Friedman DI, Liu J, et al. (2015) RNAi Interrogation of Dietary Modulation of Development, Metabolism, Behavior, and Aging in C. elegans. Cell Rep 11: 1123–1133. pmid:25959815
- 46. Rastogi S, Borgo B, Pazdernik N, Fox P, Mardis ER, et al. (2015) Caenorhabditis elegans glp-4 Encodes a Valyl Aminoacyl tRNA Synthetase. G3 (Bethesda) 5: 2719–2728.
- 47. Beanan MJ, Strome S (1992) Characterization of a germ-line proliferation mutation in C. elegans. Development 116: 755–766. pmid:1289064
- 48. Austin J, Kimble J (1987) glp-1 is required in the germ line for regulation of the decision between mitosis and meiosis in C. elegans. Cell 51: 589–599. pmid:3677168
- 49. Kodoyianni V, Maine EM, Kimble J (1992) Molecular basis of loss-of-function mutations in the glp-1 gene of Caenorhabditis elegans. Mol Biol Cell 3: 1199–1213. pmid:1457827
- 50. Hsin H, Kenyon C (1999) Signals from the reproductive system regulate the lifespan of C. elegans. Nature 399: 362–366. pmid:10360574
- 51. Lin K, Hsin H, Libina N, Kenyon C (2001) Regulation of the Caenorhabditis elegans longevity protein DAF-16 by insulin/IGF-1 and germline signaling. Nat Genet 28: 139–145. pmid:11381260
- 52. Li J, Cai T, Wu P, Cui Z, Chen X, et al. (2009) Proteomic analysis of mitochondria from Caenorhabditis elegans. Proteomics 9: 4539–4553. pmid:19670372
- 53. Venkatesan R, Sah-Teli SK, Awoniyi LO, Jiang G, Prus P, et al. (2014) Insights into mitochondrial fatty acid synthesis from the structure of heterotetrameric 3-ketoacyl-ACP reductase/3R-hydroxyacyl-CoA dehydrogenase. Nat Commun 5: 4805. pmid:25203508
- 54. Van Gilst MR, Hadjivassiliou H, Jolly A, Yamamoto KR (2005) Nuclear hormone receptor NHR-49 controls fat consumption and fatty acid composition in C. elegans. PLoS Biol 3: e53. pmid:15719061
- 55. Yoneda T, Benedetti C, Urano F, Clark SG, Harding HP, et al. (2004) Compartment-specific perturbation of protein handling activates genes encoding mitochondrial chaperones. J Cell Sci 117: 4055–4066. pmid:15280428
- 56. Prokisch H, Andreoli C, Ahting U, Heiss K, Ruepp A, et al. (2006) MitoP2: the mitochondrial proteome database—now including mouse data. Nucleic Acids Res 34: D705–711. pmid:16381964
- 57. Benedetti C, Haynes CM, Yang Y, Harding HP, Ron D (2006) Ubiquitin-like protein 5 positively regulates chaperone gene expression in the mitochondrial unfolded protein response. Genetics 174: 229–239. pmid:16816413
- 58. Haynes CM, Petrova K, Benedetti C, Yang Y, Ron D (2007) ClpP mediates activation of a mitochondrial unfolded protein response in C. elegans. Dev Cell 13: 467–480. pmid:17925224
- 59. Bugger H, Abel ED (2008) Molecular mechanisms for myocardial mitochondrial dysfunction in the metabolic syndrome. Clin Sci (Lond) 114: 195–210.
- 60. Stadtman ER, Overath P, Eggerer H, Lynen F (1960) The role of biotin and vitamin B12 coenzyme in propionate metabolism. Biochem Biophys Res Commun 2: 1–7. pmid:13833574
- 61. Rieusset J (2015) Contribution of mitochondria and endoplasmic reticulum dysfunction in insulin resistance: Distinct or interrelated roles? Diabetes Metab 41: 358–368. pmid:25797073
- 62. Liesa M, Shirihai OS (2013) Mitochondrial dynamics in the regulation of nutrient utilization and energy expenditure. Cell Metab 17: 491–506. pmid:23562075
- 63. Yang W, Hekimi S (2010) Two modes of mitochondrial dysfunction lead independently to lifespan extension in Caenorhabditis elegans. Aging Cell 9: 433–447. pmid:20346072
- 64. Luz AL, Lagido C, Hirschey MD, Meyer JN (2016) In Vivo Determination of Mitochondrial Function Using Luciferase-Expressing Caenorhabditis elegans: Contribution of Oxidative Phosphorylation, Glycolysis, and Fatty Acid Oxidation to Toxicant-Induced Dysfunction. Curr Protoc Toxicol 69: 25 28 21–25 28 22.
- 65. Bassford PJ Jr., Bradbeer C, Kadner RJ, Schnaitman CA (1976) Transport of vitamin B12 in tonB mutants of Escherichia coli. J Bacteriol 128: 242–247. pmid:135755
- 66. Kadner RJ (1990) Vitamin B12 transport in Escherichia coli: energy coupling between membranes. Mol Microbiol 4: 2027–2033. pmid:2089218
- 67. Baba T, Ara T, Hasegawa M, Takai Y, Okumura Y, et al. (2006) Construction of Escherichia coli K-12 in-frame, single-gene knockout mutants: the Keio collection. Mol Syst Biol 2: 2006 0008.
- 68. Noinaj N, Guillier M, Barnard TJ, Buchanan SK (2010) TonB-dependent transporters: regulation, structure, and function. Annu Rev Microbiol 64: 43–60. pmid:20420522
- 69. Hancock RW, Braun V (1976) Nature of the energy requirement for the irreversible adsorption of bacteriophages T1 and phi80 to Escherichia coli. J Bacteriol 125: 409–415. pmid:128553
- 70. Krewulak KD, Vogel HJ (2011) TonB or not TonB: is that the question? Biochem Cell Biol 89: 87–97. pmid:21455261
- 71. Li GW, Burkhardt D, Gross C, Weissman JS (2014) Quantifying absolute protein synthesis rates reveals principles underlying allocation of cellular resources. Cell 157: 624–635. pmid:24766808
- 72. Papp B, Pal C, Hurst LD (2003) Dosage sensitivity and the evolution of gene families in yeast. Nature 424: 194–197. pmid:12853957
- 73. Veitia RA, Bottani S, Birchler JA (2008) Cellular reactions to gene dosage imbalance: genomic, transcriptomic and proteomic effects. Trends Genet 24: 390–397. pmid:18585818
- 74. Yilmaz LS, Walhout AJ (2014) Worms, bacteria, and micronutrients: an elegant model of our diet. Trends Genet 30: 496–503. pmid:25172020
- 75. Mottram L, Speak AO, Selek RM, Cambridge EL, McIntyre Z, et al. (2016) Infection Susceptibility in Gastric Intrinsic Factor (Vitamin B12)-Defective Mice Is Subject to Maternal Influences. MBio 7.
- 76. Henriquez H, el Din A, Ozand PT, Subramanyam SB, al Gain SI (1994) Emergency presentations of patients with methylmalonic acidemia, propionic acidemia and branched chain amino acidemia (MSUD). Brain Dev 16 Suppl: 86–93.
- 77. Chi C, Ronai D, Than MT, Walker CJ, Sewell AK, et al. (2016) Nucleotide levels regulate germline proliferation through modulating GLP-1/Notch signaling in C. elegans. Genes Dev 30: 307–320. pmid:26833730
- 78. Soukas AA, Kane EA, Carr CE, Melo JA, Ruvkun G (2009) Rictor/TORC2 regulates fat metabolism, feeding, growth, and life span in Caenorhabditis elegans. Genes Dev 23: 496–511. pmid:19240135
- 79. Yen CA, Curran SP (2016) Gene-diet interactions and aging in C. elegans. Exp Gerontol 86: 106–112. pmid:26924670
- 80. Stiernagle T (2006) Maintenance of C. elegans. WormBook: 1–11.
- 81. Luz AL, Lagido C, Hirschey MD, Meyer JN (2016) In Vivo Determination of Mitochondrial Function Using Luciferase-Expressing Caenorhabditis elegans: Contribution of Oxidative Phosphorylation, Glycolysis, and Fatty Acid Oxidation to Toxicant-Induced Dysfunction. Curr Protoc Toxicol 69: 25.28.21–25.28.22.
- 82. Chung HS, Raetz CR (2010) Interchangeable domains in the Kdo transferases of Escherichia coli and Haemophilus influenzae. Biochemistry 49: 4126–4137. pmid:20394418
- 83. Rahme LG, Stevens EJ, Wolfort SF, Shao J, Tompkins RG, et al. (1995) Common virulence factors for bacterial pathogenicity in plants and animals. Science 268: 1899–1902. pmid:7604262
- 84. Garsin DA, Sifri CD, Mylonakis E, Qin X, Singh KV, et al. (2001) A simple model host for identifying Gram-positive virulence factors. Proc Natl Acad Sci U S A 98: 10892–10897. pmid:11535834
- 85. Qi B, Kniazeva M, Han M (2017) A vitamin-B2-sensing mechanism that regulates gut protease activity to impact animal's food behavior and growth. Elife 6.
- 86. Kirienko NV, Fay DS (2010) SLR-2 and JMJC-1 regulate an evolutionarily conserved stress-response network. EMBO J 29: 727–739. pmid:20057358
- 87. Bratic I, Hench J, Henriksson J, Antebi A, Burglin TR, et al. (2009) Mitochondrial DNA level, but not active replicase, is essential for Caenorhabditis elegans development. Nucleic Acids Res 37: 1817–1828. pmid:19181702
- 88. Zhou K, Zhou L, Lim Q, Zou R, Stephanopoulos G, et al. (2011) Novel reference genes for quantifying transcriptional responses of Escherichia coli to protein overexpression by quantitative PCR. BMC Mol Biol 12: 18. pmid:21513543