PMCCPMCCPMCC

Search tips
Search criteria 

Advanced

 
Logo of nihpaAbout Author manuscriptsSubmit a manuscriptHHS Public Access; Author Manuscript; Accepted for publication in peer reviewed journal;
 
Science. Author manuscript; available in PMC 2009 October 12.
Published in final edited form as:
PMCID: PMC2760269
NIHMSID: NIHMS132282

Fat Metabolism Links Germline Stem Cells and Longevity in C. elegans

Summary

Fat metabolism, reproduction, and aging are intertwined regulatory axes; however, the mechanism by which they are coupled remains poorly understood. We found that germline stem cells (GSCs) actively modulate lipid hydrolysis in Caenorhabditis elegans, which in turn regulates longevity. GSC arrest promotes systemic lipolysis via induction of a specific fat lipase. Subsequently, fat mobilization is promoted and life span is prolonged. Constitutive expression of this lipase in fat storage tissue generates lean and long-lived animals. This lipase is a key factor in the lipid hydrolysis and increased longevity that are induced by decreased insulin signaling. These results suggest a link between C. elegans fat metabolism and longevity.

Abalance of fat storage and mobilization is a universal feature of animal physiology (1). Reproduction is an energy-intensive process, which is modulated by the availability of nutrients and in turn influences lipid metabolism (2). Reproductive ability declines with age, and many organisms undergo reproductive senescence (3). Obesity increases with age and is also associated with the transition to menopause in women (4). Genetic studies have suggested endocrine roles of adipose tissue and the reproductive system in regulation of life span (58). Thus, understanding the mechanisms by which fat metabolism is coupled to reproductive cues may reveal systemic regulation of fat metabolism and provide insights into the control of aging.

In C. elegans, the energetic demands of progeny production are profound. The gonad undergoes many more mitoses than does somatic tissue, and the biomass of the oocytes produced is approximately equal to the biomass increase from egg to adult. Thus, in the absence of reproduction, a surfeit of available energy could lead to an increase in fat storage. To test this idea, we ablated the precursor cells of the germ line in C. elegans with the use of a laser microbeam. The vital dye Nile Red was used to visualize fat storage droplets in living animals (9). Opposite to the expected increase in fat storage, germ line–ablated animals stored 50% as much fat as untreated animals (Fig. 1, A to C). This finding suggested a regulatory mechanism coupling reproduction and fat metabolism.

Fig. 1
Influence of reproductive activity on fat metabolism

Fat storage is also aberrant in the sterile mutants glp-1(e2141ts) and glp-4(bn2ts), which are defective in germline proliferation (10, 11). The glp mutants showed a 50% decrease in fat storage at the nonpermissive temperature relative to the wild type (N2) (Fig. 1, D to G). A similar decrease was observed by staining with a BODIPY-labeled fatty acid analog (fig. S1) (12) or SudanBlack, a fat-specific dye (fig. S2) (13). At the permissive temperature, the glp mutants reproduced normally and their fat storage was similar to that of the wild type (fig. S3).

Fat storage can be altered by changes in either energy input or expenditure. Food intake and retention in the gut are unchanged in glp-1 (Fig. 1, H and J); the food absorption rate is also normal (Fig. 1I). Normal locomotion in glp-1 suggests that less fat storage is not due to an increase in physical activity (Fig. 1K). Therefore, decreased fat storage in the germ line–defective mutants is unlikely to be the result of alterations in energy intake and/or physical activity, and more likely reveals an altered endocrine signaling axis.

Production of vitellogenin-rich oocytes is the most energy-intensive reproductive function. We used fem-3 sterile mutants to examine whether gametogenesis influences fat storage. The gain-of-function allele fem-3(q20ts) produces only sperm, whereas the loss-of-function allele fem-3(e2006ts) produces only oocytes at the nonpermissive temperature (14, 15). Neither fem-3 mutant exhibited abnormal lipid accumulation (Fig. 2, A to D). This result excludes the possibility that gametogenesis regulates fat storage, and it also suggests that sterility per se does not cause a change in lipid accumulation.

Fig. 2
Regulation of fat metabolism by GSC proliferation

To test whether germline proliferation regulates fat storage, we shifted glp-1 mutants to the restrictive temperature at different evelopmental stages to arrest germline proliferation at distinct points. Adults that are generated from L2 (early) temperature shifts carry few mitotic germ cells, whereas adults from L4 (late) temperature shifts form the germ line with essentially wild type– sized mitotic and meiotic germ cells and differentiated sperm. Despite a very different composition of the germ line, adult fat storage was decreased to a similar extent under all conditions (Fig. 2E). One process shared by all temperature shifts is germline stem cell (GSC) arrest (16), which could induce the decrease in fat storage. We therefore shifted temperature at 1 day of adulthood, after animals started to reproduce; this should affect adult GSCs but not the already proliferated germ line. By 30 hours at the restrictive temperature, fat storage in glp-1 started to decrease (Fig. 2F). Within 48 hours, lipid accumulation in glp-1 was reduced to an extent comparable to that seen with the developmental temperature shifts (Fig. 2F). This result suggests that GSCs regulate fat storage during adulthood.

The somatic distal tip cell forms the niche of GSCs. The Notch ligand LAG-2 expressed in the distal tip cell is required to maintain GSC identity (17). Like glp-1 mutants, lag-2(q420ts) mutants (18) showed a 50% decrease in fat storage (Fig. 2G). glp-1(ar202gf) mutants with a hyperactive GLP-1, in which entry into meiosis is prevented and GSCs overproliferate (19), showed a factor of 1.7 fat increase (Fig. 2, H, I, and K), which suggests that a deficit of GSCs signals low fat storage and that GSC overproliferation signals high fat storage. No change in fat content was detected in gld-1(q485) mutants, in which early-phase meiotic germ cells reenter into the mitotic cell cycle and overproliferate (20) (Fig. 2, H, J, and K). Thus, once germ cells undergo differentiation, they lose the ability to modulate fat storage.

To understand the mechanisms by which GSCs regulate fat storage, we reduced the activities of 163 metabolic genes by RNA interference (RNAi) and screened for gene inactivations that increase fat storage in glp-1 (table S1). Among 16 potential candidate genes identified, K04A8.5 encoded a triglyceride lipase, which most strongly affected fat storage. Inactivation of K04A8.5 partially restored fat storage in glp-1 but had marginal effect on the wild type (Fig. 3A). GSC arrest caused a marked increase in the transcriptional levels of K04A8.5 (Fig. 3B), and a promoter–green fluorescent protein (GFP) reporter that was not detected under normal conditions became detectable in the glp-1 gut at the restrictive temperature (fig. S4). High gene dosage of K04A8.5 decreased fat storage in the wild type, and genetic mosaic animals showed that intestinal cells that constitutively express K04A8.5 had fewer lipid droplets than did neighboring nontransgenic cells (Fig. 3, C to E). These results imply that this lipase acts in fat storage tissue rather than in endocrine cells or GSCs. Thus, the decrease in fat storage upon GSC arrest is induced by increased lipid hydrolysis via up-regulation of K04A8.5.

Fig. 3
A role for triglyceride lipase in lipid hydrolysis and longevity

GSC arrest caused by glp-1 loss of function resulted in extended life span (Fig. 3F and table S2) (8); K04A8.5 RNAi suppressed this increased longevity but did not reduce wild-type life span (Fig. 3F and table S2). Therefore, up-regulation of this lipase gene mediates both lipid hydrolysis and longevity in GSC-arrested animals. Constitutive expression of K04A8.5 specifically in the intestine led to life spans that were 24% longer than in control siblings (Fig. 3G and table S3). Thus, lipid hydrolysis in fat storage tissue prolongs life span, which connects the metabolic functions of adipose tissue to life-span control.

We investigated the signaling pathways regulating K04A8.5 expression in the intestine. The forkhead transcription factor DAF-16 is translocated into nuclei in the intestine upon GSC arrest (21). To test whether daf-16 is involved in regulation of fat storage by GSC proliferation, we inactivated daf-16 by RNAi in wild-type and glp-1 mutants and assayed fat storage. daf-16 inactivation restored fat storage in glp-1 but did not affect wild-type fat storage (Fig. 4A and fig. S5). K04A8.5 up-regulation in glp-1 was abolished in the absence of daf-16 but was not altered in wild-type animals subjected to daf-16 RNAi (Fig. 4B). Thus, upon GSC arrest, DAF-16 is activated in the intestine to promote lipid hydrolysis through induction of K04A8.5 expression. External stresses such as heat shock and oxidative stress activate daf-16 (22, 23). After heat shock and paraquat treatment, the DAF-16 targets hsp-16.1 and ctl-2 were up-regulated but K04A8.5 was not (fig. S6). These results suggest a specific regulation of K04A8.5 by the signal from the germ line.

Fig. 4
Synergistic regulation of fat metabolism by GSC proliferation and insulin signaling

KRI-1, the human KRIT 1 homolog, and DAF-12, the nuclear hormone receptor, are both required for the intestinal nuclear localization of DAF-16 in GSC-arrested animals (21). These factors could act upstream of DAF-16 to sense signals from GSC and, in response, regulate lipid accumulation. Like daf-16 RNAi, kri-1 RNAi significantly reduced K04A8.5 expression and increased the fat content in glp-1 (Fig. 4, A and B, and fig. S5). In contrast, reducing daf-12 function did not affect K04A8.5 levels and caused a slight decrease in lipid accumulation in both wild-type and glp-1 mutants (fig. S7). Therefore, GSC arrest promotes lipid hydrolysis in the intestine through activation of the kri-1/daf-16 signaling pathway, but independently of daf-12 lipophilic hormone signaling.

We examined K04A8.5 expression in other long-lived animals, such as worms with reducing function in insulin receptor/daf-2. daf-2 is crucial in regulation of fat metabolism during larval development (24). Therefore, we reduced daf-2 function only at adulthood by RNAi feeding. Reducing daf-2 activity at adulthood caused up-regulation of K04A8.5 and decreased fat storage (Fig. 4, C and D, and fig. S8). Loss of thegerm line and reduced daf-2 signaling synergistically induced K04A8.5 and decreased fat storage (Fig. 4, C and D, and fig. S8). We also found that K04A8.5 RNAi partially suppressed the longevity of daf-2 mutants (Fig. 4E and table S4). These results suggest that lipid hydrolysis is also connected to life-span control in the daf-2 long-lived animals.

Our findings reveal an endocrine signaling axis from GSCs to fat storage tissue, with feedback from the fat storage to the longevity of the animal. Somatic stem cells are thought to mediate tissue regeneration after wounding, and such regeneration is also known to decline with aging. How the proliferation of adult stem cells is coupled to the requirement for replacement cells during normal and pathological aging may be related to the metabolic pathways we have discovered between germline stem cells and the longevity of C. elegans.

Supplementary Material

Supporting Material

Footnotes

This manuscript has been accepted for publication in Science. Please refer to the complete version of record at http://www.sciencemag.org/. The manuscript may not be reproduced or used in any manner that does not fall within the fair use provisions of the Copyright Act without the prior written permission of AAAS.

References and Notes

1. Zechner R, Strauss JG, Haemmerle G, Lass A, Zimmermann R. Curr Opin Lipidol. 2005;16:333. [PubMed]
2. Tissenbaum HA, Ruvkun G. Genetics. 1998;148:703. [PubMed]
3. Burks DJ, et al. Nature. 2000;407:377. [PubMed]
4. Carr MC. J Clin Endocrinol Metab. 2003;88:2404. [PubMed]
5. Blüher M, Kahn BB, Kahn CR. Science. 2003;299:572. [PubMed]
6. Hwangbo DS, Gershman B, Tu MP, Palmer M, Tatar M. Nature. 2004;429:562. [PubMed]
7. Giannakou ME, et al. Science. 2004;305:361. [PubMed]
8. Arantes-Oliveira N, Apfeld J, Dillin A, Kenyon C. Science. 2002;295:502. [PubMed]
9. Ashrafi K, et al. Nature. 2003;421:268. [PubMed]
10. Beanan MJ, Strome S. Development. 1992;116:755. [PubMed]
11. Priess JR, Schnabel H, Schnabel R. Cell. 1987;51:601. [PubMed]
12. Mak HY, Nelson LS, Basson M, Johnson CD, Ruvkun G. Nat Genet. 2006;38:363. [PubMed]
13. Ogg S, et al. Nature. 1997;389:994. [PubMed]
14. Hodgkin J. Genetics. 1986;114:15. [PubMed]
15. Barton MK, Schedl TB, Kimble J. Genetics. 1987;115:107. [PubMed]
16. Kimble JE, White JG. Dev Biol. 1981;81:208. [PubMed]
17. Wong MD, Jin Z, Xie T. Annu Rev Genet. 2005;39:173. [PubMed]
18. Henderson ST, Gao D, Lambie EJ, Kimble J. Development. 1994;120:2913. [PubMed]
19. Pepper AS, Killian DJ, Hubbard EJ. Genetics. 2003;163:115. [PubMed]
20. Francis R, Maine E, Schedl T. Genetics. 1995;139:607. [PubMed]
21. Berman JR, Kenyon C. Cell. 2006;124:1055. [PubMed]
22. Lee SS, Kennedy S, Tolonen AC, Ruvkun G. Science. 2003;300:644. [PubMed]
23. Wolff S, et al. Cell. 2006;124:1039. [PubMed]
24. Wolkow CA, Kimura KD, Lee MS, Ruvkun G. Science. 2000;290:147. [PubMed]
25. We thank H. Mak, J. Dittman, and J. Avruch for critical reading of the manuscript; N. Ringstad for laser ablation techniques; V. Rottiers, A. Antebi, and the Caenorhabditis Genetics Center for providing strains; A. Fire for GFP vectors; and members of the Ruvkun lab for discussions. Supported by Life Sciences Research Foundation and Ellison Medical Foundation fellowships (M.C.W.), a Human Frontier Science Program fellowship (E.J.O.), and NIH grants 5R01AG016636 and 5R37AG14161 (G.R.).