- Open Access
Methyl group donors abrogate adaptive responses to dietary restriction in C. elegans
© The Author(s) 2016
- Received: 3 December 2015
- Accepted: 14 December 2015
- Published: 17 March 2016
Almost all animals adapt to dietary restriction through alternative life history traits that affect their growth, reproduction, and survival. Economized management of fat stores is a prevalent type of such adaptations. Because one-carbon metabolism is a critical gauge of food availability, in this study, we used Caenorhabditis elegans to test whether the methyl group donor choline regulates adaptive responses to dietary restriction. We used a modest dietary restriction regimen that prolonged the fecund period without reducing the lifetime production of progeny, which is the best measure of fitness.
We found that dietary supplementation with choline abrogate the dietary restriction-induced prolongation of the reproductive period as well as the accumulation and delayed depletion of large lipid droplets and whole-fat stores and increased the survival rate in the cold. By contrast, the life span-prolonging effect of dietary restriction is not affected by choline. Moreover, we found that dietary restriction led to the enlargement of lipid droplets within embryos and enhancement of the cold tolerance of the progeny of dietarily restricted mothers. Both of these transgenerational responses to maternal dietary restriction were abrogated by exposing the parental generation to choline.
In conclusion, supplementation with the methyl group donor choline abrogates distinct responses to dietary restriction related to reproduction, utilization of fat stored in large lipid droplets, cold tolerance, and thrifty phenotypes in C. elegans.
- Dietary restriction
- Lipid droplet
- Methyl group donor
- Thrifty phenotype
- Life history traits
- C. elegans
Dietary restriction (DR) induces several adaptations, including the extension of the reproductive period, prolongation of the adult life span, and the reduction of energy turnover (Fontana and Partridge 2015). Although the life span-prolonging effect of DR and the mechanisms involved have been extensively studied in a variety of organisms, the impact of DR on the regulation of lipid droplet (LD) homeostasis is limited (Baumeier et al. 2015; Bouwman et al. 2009; Miersch and Doring 2013; Palgunow et al. 2012). LDs are evolutionarily conserved fat storage organelles containing a triacylglyceride core surrounded by a phospholipid monolayer composed mainly of phosphatidylcholine and phosphatidylethanolamine (Zhang et al. 2010b). In addition to this classical function, LDs were recently recognized to function as storage organelles for histones during embryogenesis (Cermelli et al. 2006; Li et al. 2012), assembly platforms for specific viruses (Welte 2015), and intracellular antibacterial defense systems (Anand et al. 2012). During periods of reduced food availability and/or growth, fatty acids are effectively delivered from LDs to maintain key energy-consuming processes (Barbosa et al. 2015; Lee et al. 2014; Narbonne and Roy 2009).
Functional genomic screens of the model organisms Caenorhabditis elegans and Drosophila melanogaster have been performed to identify genes that regulate LD formation and utilization (Ashrafi et al. 2003; Guo et al. 2008). These screens established that Arf1-COPI-mediated vesicular transport and the phosphatidylcholine synthesis pathway play important roles in the morphology and functionality of LDs. Many LD regulatory genes are conserved from worms to humans. Moreover, it has been shown that dietary factors, such as vaccenic acid, also regulate LD functionality (Zhang et al. 2010a). We have previously reported that in C. elegans, DR leads to the enlargement of LDs in the intestine and hypodermis (Miersch and Doring 2013; Palgunow et al. 2012), which are the main fat storage tissues of nematodes. However, little is known about the underlying cellular mechanism and the physiological role of this DR-induced LD phenotype. Because one-carbon metabolism regulates the homeostasis of phosphatidylcholine synthesis, lipogenesis, lipid droplet size, and lipolytic efficacy (Ehmke et al. 2014; Li et al. 2011), in this study, we used C. elegans to determine whether the methyl group donor choline plays a regulatory role in the enlargement of LDs and other adaptive phenotypes that are induced by DR.
Intake of the methyl group donor choline abrogates both the enlargement of intestinal lipid droplets and the increase in the fat content of dietarily restricted worms
Choline does not abrogate the enlargement of hypodermal lipid droplets induced by dietary restriction
Choline abrogates the delayed depletion of the fat stores of dietarily restricted worms
Choline abrogates the enlargement of the lipid droplets of progeny (F 1) produced by dietarily restricted mothers (P o)
Choline abrogates the increased survival rates observed in the cold in dietarily restricted worms and in the larvae produced by dietarily restricted mothers
Choline abrogates the extension of the reproductive period, but not the increase in the life span of dietarily restricted worms
The altered lipid composition, increased LD size, and higher survival rates in the cold observed in embryos derived from DR mothers might indicate that the reproduction of mothers subjected to DR is altered. As expected, DR prolonged the fecund period of the worms compared with those exposed to the AL conditions (Fig. 5d). The resulting lifetime progeny production rate, which is the best indicator of fitness, was not reduced and was even slightly increased by DR (Fig. 5e). The DR-induced extension of the reproductive period was completely abrogated by either choline or methionine supplementation (Fig. 5d). Surprisingly, the DR-mediated life span extension was only slightly reduced by choline or methionine supplementation (Fig. 5f), indicating that these methyl group donors exert specific effects on LD size, fat storage, survival in the cold, and reproduction.
Almost all organisms respond to reduced food intake, or DR, via alternative life history traits that ensure survival, growth, and reproduction. In the present study, we applied a standardized DR regime (Miersch and Doring 2013; Palgunow et al. 2012) during postembryonic development. As this DR regime prevents developmental delay and growth retardation, it mimics a moderate, but sufficient food intake. The phenotypes resulting from implementing this DR regime include the accumulation of fat in large LDs, delayed depletion of fat stores, and prolongation of the fecund period without a reduction of the lifetime progeny production rate. Thus, the observed DR-induced phenotypes are highly consistent with the life history theory. Another basic theory argues that a food-restricted mother modifies the phenotype of her progeny such that they are prepared for survival in a poor nutritional environment (Barker 2001). The enlargement of the LDs and the accumulation of triacylglycerides in embryos derived from DR mothers might represent such a thrifty phenotype, assuming that the accumulated, larger embryonic LDs are more resistant to starvation-induced depletion, as observed in the mothers.
As mentioned above, our findings regarding the DR-induced phenotypes are in good agreement with the life history theory and the thrifty phenotype theory. These types of ultimate explanations are insufficient to explain the biological functions of the phenotypes in terms of immediate physiological or environmental factors. In searching for such factors, we consider that animals with a genetic deficiency in methyl group donors phenocopies the observed DR-induced effects. For example, C. elegans mutants deficient in the synthesis of SAM, the main methyl group donor found in most organisms, show enlarged LDs during both the adult and embryonic stages, increased fat stores, reduced levels of phosphatidylcholine, and delayed depletion of fat stores (Ehmke et al. 2014; Hansen et al. 2005; Walker et al. 2011). Several animal- and patient-based studies have suggested that a diet deficient in methyl group donors is an important factor in the etiology of non-alcoholic fat liver (Leermakers et al. 2015). For example, a choline-deficient diet causes hepatic fat accumulation (Rinella and Green 2004; Zeisel et al. 1991). We suggest that endogenous and exogenous methyl group donors are critical under DR conditions and that the resulting activity of one-carbon metabolism in turn regulates LD size and fat storage. This phenomenon is particularly true for C. elegans and other nematodes because their food source, Escerichia coli, does not contain phosphatidylcholine. Accordingly, we found that dietary supplementation with choline as well as methionine abrogates the DR-induced fat-related phenotypes. Interestingly, folic acid and vitamin B12 are also involved in determining the activity of one-carbon metabolism. Restriction of these vitamins may be related to the fat-related phenotypes observed under DR. A study in rats has shown that vitamin B12 deficiency causes increased fatty acid synthesis (Matlib et al. 1979). All of these findings support the view that one-carbon metabolism is a critical gauge of food availability and a key pathway involved in regulating the adaptive storage and utilization of fat.
The most abundant phospholipid in the LD monolayer is PC, which can be synthesized from choline (via the Kennedy pathway), or via the SAM-dependent methylation of phosphoethanolamine (in nematodes and plants) or phosphatidylethanolamine (in mammals) (Brendza et al. 2007; Palavalli et al. 2006). It has been shown that depletion of PC or loss-of-function mutations of the genes that mediate methylation-dependent PC synthesis (sams-1 and pmt-1) leads to enlargement of LDs (Bartz et al. 2007; Guo et al. 2008; Szymanski et al. 2007; Walker et al. 2011). Further studies revealed that LD enlargement occurs when there is a reduced level of PC due to fusion of the existing LDs (Guo et al. 2008; Krahmer et al. 2011; Li et al. 2011; Walker et al. 2011). Based on these findings, we propose that the expansion of LDs induced by DR is caused by the decreased availability of methyl group donors and subsequent reduction of PC levels, which in turn promotes LD fusion. This hypothesis is supported by the observation that dietary supplementation with the methyl group donors choline and methionine increases the PC content and decreases LD size in DR worms.
Remarkably, embryos derived from DR mothers also exhibit a decreased PC content and very large LDs. Both of these phenotypes can be abolished by choline or methionine supplementation of the restricted diet of the mothers, indicating that these methyl group donors are provided to the embryos maternally. Consistent with this conclusion, the embryos of a methyl group donor-deficient mutant (sams-1) also exhibit large LDs. As enlarged embryonic LDs as well as cold tolerance are also observed in DR mother-derived L1/2 larvae, we suggest that the maternally provided methyl group donors persist in the progeny. Thus, the existence of a relationship between the availability of methyl group donors, PC contents, and LD size provides an explanation for the observed DR-induced fat-related phenotypes and their abolishment through choline or methionine supplementation. As the reduced PC content, increased LD size, and adaptation to cold are inherited by the next generation and can be abolished by supplementation with methyl group donors, the one-carbon metabolism of the mothers may play an important role in the occurrence of these thrifty phenotypes. Nevertheless, we cannot exclude that the inherited effect has something to do with histone methylation and subsequent gene expression. This should be studied in future experiments focusing on epigenetic effects.
We found that the starvation-induced depletion of fat stores, particularly that of the large LDs, is reduced in DR worms. This fat-sparing effect can also be abolished by supplementation with methyl group donors. In Drosophila, it has been shown that DR increases starvation resistance (Burger et al. 2007). Because the surface-to-volume ratio is lower in larger LDs than in smaller LDs, the rate of degradation of the former by lipases might be decreased. Consistent with this hypothesis, a C. elegans mutant (dhs-28) deficient in peroxisomal β-oxidation is characterized by extremely large LDs that are more resistant to lipase-mediated lipolysis compared with smaller LDs (Zhang et al. 2010a). Moreover, studies in flies have shown that the large LDs that form due to reduced PC levels are more resistant to lipolysis (Guo et al. 2008; Krahmer et al. 2011). In mutant mice, the generation of small LDs leads to enhanced lipolysis (Nishino et al. 2008). The size of LDs is functionally important in the supply of fatty acids. From this point of view, a decreased rate of supply of fatty acids derived from large LDs may contribute to the prolonged reproductive period of DR worms. This hypothesis should be tested in future studies using mutants that are not responsive to starvation-induced fat depletion.
We have demonstrated that subjecting C. elegans to a moderate DR regime during the postembryonic period induces the prolongation of the reproductive period, the accumulation and delayed depletion of large LDs and whole-fat stores, an increased survival rate in the cold, the enlargement of LDs, and a higher level of cold resistance in the filial generation. Because all of these effects are prevented by dietary supplementation with methyl group donors, we conclude that one-carbon metabolism is a critical gauge of food availability, a key pathway in regulating the adaptive storage and utilization of fat, and an important determinant for the induction of thrifty phenotypes.
Worm strains, culture, dietary restriction
The wild-type strain used in this study was Bristol N2. A VS20 strain expressing an ATGL-1::GFP fusion protein [atgl-1p::atgl-1::GFP] was used as a lipid droplet reporter strain. The strain pwls[vit-2p::vit-2::GFP] was used for the visualization of vitellogenin-containing yolk granules. The worms were cultured at 20 °C on nematode growth medium (NGM) plates using E. coli OP50 as the food source, following standard methods (Brenner 1974). For the supplementation experiments, solutions of choline (10 mM), ethanolamine (10 mM), betaine (10 mM), or methionine (1 mM) were spread on the bacterial lawn. Age synchronization of the nematodes was achieved through hypochlorite treatment of gravid adults. Dietary restriction of the worms was achieved as previously described (Palgunow et al. 2012). In short, adjusted optical densities (250 μl, OD600 0.7 or 1.5) of the E. coli strain OP50 were spread onto antibiotic-free agar plates (without peptone) and incubated for 16 h at 37 °C. This leads to different amounts of bacteria per agar plate depending on the OD of seeded OP50. To further standardize food availability per worm, 500 synchronized embryos were sorted onto AL and dDR agar plates by flow cytometry and were cultivated at 20 °C until reaching the L4 or adult stage. To exclude starvation, L4 larvae and adult worms were transferred daily to fresh agar plates.
Number of progeny and reproductive period
To determine the number of progeny, 48 h after synchronization and cultivation under a particular condition, L4 larvae were placed on plates containing a ring of palmitic acid to prevent their escape. Five worms per plate were cultivated for an additional 48 h. This time point was considered day 1 of adulthood and progeny production. The animals were subsequently transferred to new plates at 24-h intervals until the end of their reproductive period. The progeny on the residual plates were counted the day after the adults were transferred. Three plates were analyzed for each condition in three independent experiments. The reproductive period was calculated as the period during which 95 % of the progeny were produced.
Survival rate under cold conditions
Immediately before the worms were shifted to 0 °C, the NGM plates were divided into four segments that were placed in different positions in the incubator. The nematodes were transferred to 0 °C as larvae or young adults, and survival was monitored at specific time points. The samples were analyzed in triplicate for each condition and time point. The survival rate was calculated as the percentage of dead individuals after 24 h of recovery at 20 °C among the total number of worms that had been counted immediately after incubation at 0 °C. Worms were scored as dead if they did not respond when gently touched with a platinum wire.
Synchronized worms were grown for 48 h on NGM agar plates until reaching the L4 stage. Approximately 4000 worms were harvested from 10 to 12 NGM plates/condition and were washed three times with M9 buffer. Control worms (0 h of starvation) with or without choline supplementation were immediately sorted using a COPAS Biosort flow cytometric system into Precellys vials (1000 worms/sample) and were stored at −80 °C until further processing. To induce starvation, worms were cultivated in 15-ml Falcon tubes in a Nutator mixer in 3 ml of M9 buffer supplemented with an antibiotic (dilution: 1:100, Cell Culture Guard, AppliChem) and choline or the vehicle (H2O). After 24 and 72 h of starvation, the worms were collected as described above for the control worms (0 h of starvation). The samples were used for TLC and protein quantification. An aliquot of live worms grown under each condition (0, 24, or 72 h of starvation) was subjected to vital BODIPY™ 493/503 staining for analysis of the number and size of the lipid droplets.
BODIPY™ 493/503 vital staining and fluorescence imaging
To visualize fat storage in worms and embryos, vital BODIPY™ 493/503 (Invitrogen, Darmstadt, Germany) staining was performed as previously described (Klapper et al. 2011). Briefly, freshly harvested worms were washed three times with M9 buffer and were incubated in 500 μL of BODIPY™ 493/503 solution (6.7 μg/μl in M9 buffer) for 20 min. After washing twice with M9, the worms were anesthetized using sodium azide (1 %) and immediately examined via microscopy. BODIPY™ 493/503 fluorescence was visualized using an Axio Imager system and a Z1 microscope equipped with a 38 HE filter (excitation: BP 470/40, beam splitter: FT 495, emission: BP 525/50), coupled to an apotome-sectioning system (ApoTome.2, Zeiss). To distinguish between BODIPY™ 493/503-positive structures and auto-fluorescent lysosome-related organelles, auto-fluorescence was imaged using the DAPI channel. GFP fluorescence was visualized with a 38 HE filter (excitation BP 470/40; beam splitter FT 495; emission BP 525/50).
Analysis of the number and size of lipid droplets
BODIPY™ 493/503-stained lipid droplets localized in selected regions were imaged via 3D fluorescence microscopy using an Axio Imager Z1 microscope and a Plan-Apochromat ×63/1.3 oil immersion objective. The apotome-sectioning system was used to collect z-stacks with a step size of 0.5 μm. The z-stacks comprised 21 planar images (format, 138.4 × 104 μm; 692 × 520 pixels). Images were captured using an AxioCam MRm (Zeiss) system. ImageJ software (version 1.47 h) and the 3D spot segmentation plug-in were used to analyze the z-stacks. BODIPY™ 493/503-positive structures were automatically identified, and the volume of each droplet was evaluated by totaling the number of voxels per droplet. If necessary, the brightness and contrast levels were manually adjusted before performing the calculations.
After thawing worms stored at −80 °C, worms collected using the COPAS Biosort system were analyzed by thin-layer chromatography (Matyash et al. 2008). Lipids were extracted from 1000 or 2000 homogenized worms (Precellys24 homogenizer; full speed; 3 × 10 s) using a solution containing 375 μl of methanol, 1250 μl of methyl-tert-butyl-ether , and 312 μl of H2O (3:10:2.5 [v]) and were dissolved in 30 μl of chloroform. Probes were applied to Polygram SIL G pre-coated TLC sheets (20 × 20 cm; 0.2-mm silica gel; Macherey-Nagel) using hexane/diethyl-ether/formic acid (20:20:1 [v]) as the mobile phase for TAG and phospholipids. A 5-μl aliquot of worm extract was applied to each lane to ensure that the amounts of TAGs and phospholipids were within the linear range of the standard curves. The assays were conducted in duplicate. The lipid spots were stained for 20 s in a dip solution containing 10 % copper (II) sulfate, 8 % phosphor acid, and 5 % methanol. Quantification was achieved by calculating the spot intensity per area (pixel/μm2) using AlphaEaseFC (BioRad) software. Triolein (Sigma Aldrich, Germany) and a phospholipid mixture (Sigma Aldrich, P3817) were used as standards. All of the results are presented as the mean values for the standard and diluted probes.
Lipid composition analysis
Embryos were washed three times with M9 buffer supplemented with Tween 20 (1:100,000) to prevent the embryos from attaching to the tubes. Defined numbers of embryos that were sorted using the COPAS Biosort system were then transferred to chloroform-rinsed Pyrex tubes and were immediately frozen at −80 °C until being utilized for mass spectroscopy. The contents of the fatty acids triacylglyceride, phosphatidylcholine, and plasmalogen were analyzed using a high-resolution LC-MS/MS platform (Fauland et al. 2011) equipped with a Lipid Data Analyzer (Hartler et al. 2011). The results were normalized according to the contents of different fatty acid classes, the sample weight, and the protein content.
Statistical analysis was performed using Microsoft Excel (2003) and GraphPad Prism (Version 4.0) software. Unless otherwise noted, the data represent the mean ± SEM of at least three independent experiments. The significance of the differences was calculated using an unpaired two-tailed t test. Welch’s correction was applied if the variances were different. Differences were considered significant at p < 0.05 (*), p < 0.01 (**), and p < 0.001 (***).
We thank Astrid Reinke and Fabian Neumann for high throughput processing of plates and reagents. The study was funded by the University of Kiel and the leisure time of the authors.
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- Anand P, Cermelli S, Li Z, Kassan A, Bosch M, Sigua R, Huang L, Ouellette AJ, Pol A, Welte MA, Gross SP (2012) A novel role for lipid droplets in the organismal antibacterial response. eLife 1:e00003. doi:10.7554/eLife.00003 View ArticlePubMedPubMed CentralGoogle Scholar
- Ashrafi K, Chang FY, Watts JL, Fraser AG, Kamath RS, Ahringer J, Ruvkun G (2003) Genome-wide RNAi analysis of Caenorhabditis elegans fat regulatory genes. Nature 421(6920):268–272View ArticlePubMedGoogle Scholar
- Barbosa AD, Savage DB, Siniossoglou S (2015) Lipid droplet-organelle interactions: emerging roles in lipid metabolism. Curr Opin Cell Biol 35:91–97. doi:10.1016/j.ceb.2015.04.017 View ArticlePubMedGoogle Scholar
- Barker DJP (2001) Type 2 diabetes: the thrifty phenotype—preface. Br Med Bull 60:1–3. doi:10.1093/Bmb/60.1.1 View ArticleGoogle Scholar
- Bartz R, Li WH, Venables B, Zehmer JK, Roth MR, Welti R, Anderson RG, Liu P, Chapman KD (2007) Lipidomics reveals that adiposomes store ether lipids and mediate phospholipid traffic. J Lipid Res 48(4):837–847View ArticlePubMedGoogle Scholar
- Baumeier C, Kaiser D, Heeren J, Scheja L, John C, Weise C, Eravci M, Lagerpusch M, Schulze G, Joost HG, Schwenk RW, Schurmann A (2015) Caloric restriction and intermittent fasting alter hepatic lipid droplet proteome and diacylglycerol species and prevent diabetes in NZO mice. Biochim Biophys Acta 1851(5):566–576. doi:10.1016/j.bbalip.2015.01.013 View ArticlePubMedGoogle Scholar
- Bouwman FG, Claessens M, van Baak MA, Noben JP, Wang P, Saris WH, Mariman EC (2009) The physiologic effects of caloric restriction are reflected in the in vivo adipocyte-enriched proteome of overweight/obese subjects. J Proteome Res 8(12):5532–5540. doi:10.1021/pr900606m View ArticlePubMedGoogle Scholar
- Brendza KM, Haakenson W, Cahoon RE, Hicks LM, Palavalli LH, Chiapelli BJ, McLaird M, McCarter JP, Williams DJ, Hresko MC, Jez JM (2007) Phosphoethanolamine N-methyltransferase (PMT-1) catalyses the first reaction of a new pathway for phosphocholine biosynthesis in Caenorhabditis elegans. Biochem J 404(3):439–448. doi:10.1042/BJ20061815 View ArticlePubMedPubMed CentralGoogle Scholar
- Brenner S (1974) The genetics of Caenorhabditis elegans. Genetics 77(1):71–94PubMedPubMed CentralGoogle Scholar
- Burger JM, Hwangbo DS, Corby-Harris V, Promislow DE (2007) The functional costs and benefits of dietary restriction in Drosophila. Aging Cell 6(1):63–71. doi:10.1111/j.1474-9726.2006.00261.x View ArticlePubMedGoogle Scholar
- Cermelli S, Guo Y, Gross SP, Welte MA (2006) The lipid-droplet proteome reveals that droplets are a protein-storage depot. Curr Biol 16(18):1783–1795. doi:10.1016/j.cub.2006.07.062 View ArticlePubMedGoogle Scholar
- Ehmke M, Luthe K, Schnabel R, Doring F (2014) S-Adenosyl methionine synthetase 1 limits fat storage in Caenorhabditis elegans. Genes Nutr 9(2):386. doi:10.1007/s12263-014-0386-6 View ArticlePubMedPubMed CentralGoogle Scholar
- Fauland A, Kofeler H, Trotzmuller M, Knopf A, Hartler J, Eberl A, Chitraju C, Lankmayr E, Spener F (2011) A comprehensive method for lipid profiling by liquid chromatography-ion cyclotron resonance mass spectrometry. J Lipid Res 52(12):2314–2322. doi:10.1194/jlr.D016550 View ArticlePubMedPubMed CentralGoogle Scholar
- Fontana L, Partridge L (2015) Promoting health and longevity through diet: from model organisms to humans. Cell 161(1):106–118. doi:10.1016/j.cell.2015.02.020 View ArticlePubMedGoogle Scholar
- Guo Y, Walther TC, Rao M, Stuurman N, Goshima G, Terayama K, Wong JS, Vale RD, Walter P, Farese RV (2008) Functional genomic screen reveals genes involved in lipid-droplet formation and utilization. Nature 453(7195):657–661. doi:10.1038/nature06928 View ArticlePubMedPubMed CentralGoogle Scholar
- Hansen M, Hsu AL, Dillin A, Kenyon C (2005) New genes tied to endocrine, metabolic, and dietary regulation of lifespan from a Caenorhabditis elegans genomic RNAi screen. PLoS Genet 1(1):119–128. doi:10.1371/journal.pgen.0010017 View ArticlePubMedGoogle Scholar
- Hartler J, Trotzmuller M, Chitraju C, Spener F, Kofeler HC, Thallinger GG (2011) Lipid data analyzer: unattended identification and quantitation of lipids in LC-MS data. Bioinformatics 27(4):572–577. doi:10.1093/bioinformatics/btq699 View ArticlePubMedGoogle Scholar
- Klapper M, Ehmke M, Palgunow D, Bohme M, Matthaus C, Bergner G, Dietzek B, Popp J, Doring F (2011) Fluorescence-based fixative and vital staining of lipid droplets in Caenorhabditis elegans reveal fat stores using microscopy and flow cytometry approaches. J Lipid Res 52(6):1281–1293. doi:10.1194/jlr.D011940 View ArticlePubMedPubMed CentralGoogle Scholar
- Krahmer N, Guo Y, Wilfling F, Hilger M, Lingrell S, Heger K, Newman HW, Schmidt-Supprian M, Vance DE, Mann M, Farese RV Jr, Walther TC (2011) Phosphatidylcholine synthesis for lipid droplet expansion is mediated by localized activation of CTP:phosphocholine cytidylyltransferase. Cell Metab 14(4):504–515. doi:10.1016/j.cmet.2011.07.013 View ArticlePubMedPubMed CentralGoogle Scholar
- Lee JH, Kong J, Jang JY, Han JS, Ji Y, Lee J, Kim JB (2014) Lipid droplet protein LID-1 mediates ATGL-1-dependent lipolysis during fasting in Caenorhabditis elegans. Mol Cell Biol 34(22):4165–4176. doi:10.1128/MCB.00722-14 View ArticlePubMedPubMed CentralGoogle Scholar
- Leermakers ET, Moreira EM, Kiefte-de Jong JC, Darweesh SK, Visser T, Voortman T, Bautista PK, Chowdhury R, Gorman D, Bramer WM, Felix JF, Franco OH (2015) Effects of choline on health across the life course: a systematic review. Nutr Rev 73(8):500–522. doi:10.1093/nutrit/nuv010 View ArticlePubMedGoogle Scholar
- Li Y, Na K, Lee HJ, Lee EY, Paik YK (2011) Contribution of sams-1 and pmt-1 to lipid homoeostasis in adult Caenorhabditis elegans. J Biochem 149(5):529–538. doi:10.1093/jb/mvr025 View ArticlePubMedGoogle Scholar
- Li Z, Thiel K, Thul PJ, Beller M, Kuhnlein RP, Welte MA (2012) Lipid droplets control the maternal histone supply of Drosophila embryos. Curr Biol 22(22):2104–2113. doi:10.1016/j.cub.2012.09.018 View ArticlePubMedPubMed CentralGoogle Scholar
- Matlib MA, Frenkel EP, Mukherjee A, Henslee J, Srere PA (1979) Enzymatic properties of mitochondria isolated from normal and vitamin B12-deficient rats. Arch Biochem Biophys 197(2):388–395View ArticlePubMedGoogle Scholar
- Matyash V, Liebisch G, Kurzchalia TV, Shevchenko A, Schwudke D (2008) Lipid extraction by methyl-tert-butyl ether for high-throughput lipidomics. J Lipid Res 49(5):1137–1146. doi:10.1194/jlr.D700041-JLR200 View ArticlePubMedPubMed CentralGoogle Scholar
- Miersch C, Doring F (2013) Sex differences in body composition, fat storage, and gene expression profile in Caenorhabditis elegans in response to dietary restriction. Physiol Genomics 45(13):539–551. doi:10.1152/physiolgenomics.00007.2013 View ArticlePubMedGoogle Scholar
- Narbonne P, Roy R (2009) Caenorhabditis elegans dauers need LKB1/AMPK to ration lipid reserves and ensure long-term survival. Nature 457(7226):210–214. doi:10.1038/nature07536 View ArticlePubMedGoogle Scholar
- Nishino N, Tamori Y, Tateya S, Kawaguchi T, Shibakusa T, Mizunoya W, Inoue K, Kitazawa R, Kitazawa S, Matsuki Y, Hiramatsu R, Masubuchi S, Omachi A, Kimura K, Saito M, Amo T, Ohta S, Yamaguchi T, Osumi T, Cheng J, Fujimoto T, Nakao H, Nakao K, Aiba A, Okamura H, Fushiki T, Kasuga M (2008) FSP27 contributes to efficient energy storage in murine white adipocytes by promoting the formation of unilocular lipid droplets. J Clin Invest 118(8):2808–2821. doi:10.1172/JCI34090 PubMedPubMed CentralGoogle Scholar
- Palavalli LH, Brendza KM, Haakenson W, Cahoon RE, McLaird M, Hicks LM, McCarter JP, Williams DJ, Hresko MC, Jez JM (2006) Defining the role of phosphomethylethanolamine N-methyltransferase from Caenorhabditis elegans in phosphocholine biosynthesis by biochemical and kinetic analysis. Biochemistry 45(19):6056–6065. doi:10.1021/bi060199d View ArticlePubMedGoogle Scholar
- Palgunow D, Klapper M, Doring F (2012) Dietary restriction during development enlarges intestinal and hypodermal lipid droplets in Caenorhabditis elegans. PLoS One 7(11):e46198. doi:10.1371/journal.pone.0046198 View ArticlePubMedPubMed CentralGoogle Scholar
- Rinella ME, Green RM (2004) The methionine-choline deficient dietary model of steatohepatitis does not exhibit insulin resistance. J Hepatol 40(1):47–51View ArticlePubMedGoogle Scholar
- Szymanski KM, Binns D, Bartz R, Grishin NV, Li WP, Agarwal AK, Garg A, Anderson RG, Goodman JM (2007) The lipodystrophy protein seipin is found at endoplasmic reticulum lipid droplet junctions and is important for droplet morphology. Proc Natl Acad Sci USA 104(52):20890–20895View ArticlePubMedPubMed CentralGoogle Scholar
- Walker AK, Jacobs RL, Watts JL, Rottiers V, Jiang K, Finnegan DM, Shioda T, Hansen M, Yang F, Niebergall LJ, Vance DE, Tzoneva M, Hart AC, Naar AM (2011) A conserved SREBP-1/phosphatidylcholine feedback circuit regulates lipogenesis in metazoans. Cell 147(4):840–852. doi:10.1016/j.cell.2011.09.045 View ArticlePubMedPubMed CentralGoogle Scholar
- Welte MA (2015) Expanding roles for lipid droplets. Curr Biol 25(11):R470–R481. doi:10.1016/j.cub.2015.04.004 View ArticlePubMedGoogle Scholar
- Zeisel SH, Da Costa KA, Franklin PD, Alexander EA, Lamont JT, Sheard NF, Beiser A (1991) Choline, an essential nutrient for humans. FASEB J 5(7):2093–2098PubMedGoogle Scholar
- Zhang SO, Box AC, Xu N, Le Men J, Yu J, Guo F, Trimble R, Mak HY (2010a) Genetic and dietary regulation of lipid droplet expansion in Caenorhabditis elegans. Proc Natl Acad Sci U S A 107(10):4640–4645. doi:10.1073/pnas.0912308107 View ArticlePubMedPubMed CentralGoogle Scholar
- Zhang SO, Trimble R, Guo F, Mak HY (2010b) Lipid droplets as ubiquitous fat storage organelles in C. elegans. BMC Cell Biol 11:96. doi:10.1186/1471-2121-11-96 View ArticlePubMedPubMed CentralGoogle Scholar