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Characterization of N-Acyl Phosphatidylethanolamine-Specific Phospholipase-D Isoforms in the Nematode Caenorhabditis elegans

  • Neale Harrison,

    Current address: School of Biosciences, University of Birmingham, Birmingham, United Kingdom

    Affiliation Department of Metabolism & Aging, The Scripps Research Institute, Scripps Florida, Jupiter, Florida, United States of America

  • Museer A. Lone,

    Affiliation Department of Metabolism & Aging, The Scripps Research Institute, Scripps Florida, Jupiter, Florida, United States of America

  • Tiffany K. Kaul,

    Affiliation Department of Metabolism & Aging, The Scripps Research Institute, Scripps Florida, Jupiter, Florida, United States of America

  • Pedro Reis Rodrigues,

    Affiliation Department of Metabolism & Aging, The Scripps Research Institute, Scripps Florida, Jupiter, Florida, United States of America

  • Ifedayo Victor Ogungbe,

    Current address: Department of Chemistry & Biochemistry, Jackson State University, Jackson, Mississippi, United States of America

    Affiliation Department of Metabolism & Aging, The Scripps Research Institute, Scripps Florida, Jupiter, Florida, United States of America

  • Matthew S. Gill

    mgill@scripps.edu

    Affiliation Department of Metabolism & Aging, The Scripps Research Institute, Scripps Florida, Jupiter, Florida, United States of America

Characterization of N-Acyl Phosphatidylethanolamine-Specific Phospholipase-D Isoforms in the Nematode Caenorhabditis elegans

  • Neale Harrison, 
  • Museer A. Lone, 
  • Tiffany K. Kaul, 
  • Pedro Reis Rodrigues, 
  • Ifedayo Victor Ogungbe, 
  • Matthew S. Gill
PLOS
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Abstract

N-acylethanolamines are an important class of lipid signaling molecules found in many species, including the nematode Caenorhabditis elegans (C. elegans) where they are involved in development and adult lifespan. In mammals, the relative activity of the biosynthetic enzyme N-acyl phosphatidylethanolamine-specific phospholipase-D and the hydrolytic enzyme fatty acid amide hydrolase determine N-acylethanolamine levels. C. elegans has two N-acyl phosphatidylethanolamine-specific phospholipase-D orthologs, nape-1 and nape-2, that are likely to have arisen from a gene duplication event. Here, we find that recombinant C. elegans NAPE-1 and NAPE-2 are capable of generating N-acylethanolamines in vitro, confirming their functional conservation. In vivo, they exhibit overlapping expression in the pharynx and the nervous system, but are also expressed discretely in these and other tissues, suggesting divergent roles. Indeed, nape-1 over-expression results in delayed growth and shortened lifespan only at 25°C, while nape-2 over-expression results in significant larval arrest and increased adult lifespan at 15°C. Interestingly, deletion of the N-acylethanolamine degradation enzyme faah-1 exacerbates nape-1 over-expression phenotypes, but suppresses the larval arrest phenotype of nape-2 over-expression, suggesting that faah-1 is coupled to nape-2, but not nape-1, in a negative feedback loop. We also find that over-expression of either nape-1 or nape-2 significantly enhances recovery from the dauer larval stage in the insulin signaling mutant daf-2(e1368), but only nape-1 over-expression reduces daf-2 adult lifespan, consistent with increased levels of the N-acylethanolamine eicosapentaenoyl ethanolamine. These results provide evidence that N-acylethanolamine biosynthetic enzymes in C. elegans have conserved function and suggest a temperature-dependent, functional divergence between the two isoforms.

Introduction

N-acylethanolamines (NAEs) are bioactive lipids that are involved in diverse physiological processes in both animals and plants, and are composed of an acyl chain of varying length and unsaturation that is amide-linked to an ethanolamine head group [1], [2]. In mammals, the first step in the NAE biosynthetic pathway is the synthesis of N-acyl phosphatidylethanolamine (NAPE) from phosphatidylethanolamine and phosphatidylcholine, by the enzyme N-acyl transferase (NAT) [1]. Although various Ca2+ independent isoforms have been cloned and characterized, the Ca2+ dependent NAT has yet to be identified [3]. The glycerophospholipid substrates of this enzyme are abundantly found in most membranes, but levels of NAPEs are maintained at very low levels [4], suggesting that the activity of NAT represents the rate-limiting step in NAE biosynthesis. In the second step, NAEs are synthesized from their precursor NAPEs by the enzyme NAPE-specific phospholipase-D (NAPE-PLD) [5], [6]. Cloning of mammalian NAPE-PLD revealed no homology to other known PLDs, but instead indicated that it belongs to the novel zinc metallohydrolase family with a β-lactamase fold [7]. NAPE-PLD is capable of producing various medium and long chain bioactive NAEs in a Ca2+-dependent manner [7] and the enzyme is specific for NAPE substrates, with no activity towards other phospholipids [8].

Among other enzymes of the endocannabinoid metabolic pathway, sequence homologs of NAPE-PLD have been identified in many organisms [9], and NAPE-PLD has been cloned and characterized from rat, mouse and humans [7]. Consistent with the widespread function of NAEs, NAPE-PLD expression in mammals is detected in most tissues, being particularly high in brain and testis [7]. Mammalian NAPE-PLD is a membrane bound protein, localized mainly to the intracellular microsomal membranes. Due to the magnitude of physiological responses to minute changes in levels of different NAEs at the tissue and organismal level, the activity of NAPE-PLD is tightly controlled, especially at the transcriptional level [10], [11]. The enzyme activity is stimulated by Ca2+ and activation of ionotropic glutamate N-methyl-D-aspartate receptors [12], as well as by the major neurotransmitters, dopamine [13], glutamine [14] and acetylcholine [15]. In the last step of the pathway, NAE levels are then regulated by fatty acid amide hydrolase (FAAH) which hydrolyses NAEs into free fatty acids and ethanolamine [16]. Though the levels of NAEs are mostly regulated through this canonical pathway, other anabolic and catabolic enzymes have been described that modulate NAE levels [3].

Previous work from our laboratory identified the enzyme components for NAE metabolism in the free living nematode, C. elegans, as well as a set of diverse NAEs that differed in their fatty acid composition and level of unsaturation [17]. While we were able to show that NAE levels were modulated by over-expression of the C. elegans homolog of FAAH, we did not address the role of NAE biosynthetic enzymes in the worm, other than to show that one of the orthologs, nape-1, was expressed in similar tissues to faah-1 [17]. In the present work we have carried out a more detailed examination of the two C. elegans homologs of the NAE synthesizing enzyme NAPE-PLD, nape-1 and nape-2. We show that both proteins are capable of catalyzing the production of NAEs in vitro, indicating that they are functional orthologs of mammalian NAPE-PLD. We also show that despite strong sequence similarity, the function of the two homologs may have diverged and they may be responsible for temperature-dependent effects of NAEs on development and lifespan.

Materials and Methods

Chemicals

Palmitoyl ethanolamide-d4 (PEA-d4) and arachidonoyl ethanolamide-d4 (AEA-d4) were obtained from Cayman Chemical (MI). N-palmitoyl phosphatidylethanolamine (N-palmitoyl PE) was obtained from Enzo Life Sciences (PA) and N-arachidonoyl PE (1,2-dioleoyl-sn-glycero-3-phosphoethanolamine-N-arachidonoyl ammonium salt) was obtained from Avanti Polar Lipids, Inc (AL). BSTFA was from Sigma Aldrich (MO). All solvents were of gas chromatography-mass spectrometry (GC-MS) grade and all other reagents were of the highest grade available.

Cloning of nape-1 and nape-2 into the pET28a expression vector

nape-1 and nape-2 were amplified from wild type cDNA with primers containing engineered restriction sites. These fragments were T/A cloned into the pGEM-T Easy vector (Promega) and sequenced. The corresponding fragments were then cloned into the E. coli expression vector pET28a (Novagen) using the NdeI/XhoI sites for nape-1 and the XhoI/EcoRI sites for nape-2.

OverExpress C41(DE3) chemically competent cells (Lucigen) were transformed with pET28a(nape-1) or pET28a(nape-2) constructs. Recombinant polyhistidine-tagged NAPE-1 and NAPE-2 were expressed in C41(DE3) positive clones by 1 mM isopropyl-β-D-thiogalactopyranoside (IPTG) induction at an A600 of 0.6 for 4 hours at 37°C. Induced cells were pelleted at 7000× g for 20 min at 4°C, and stored overnight at −20°C. For recombinant protein purification, frozen cells were thawed and incubated on ice with 50 mM Tris buffer (pH 8.0) containing 100 mM NaCl and 0.2 mM n-dodecyl-β-D-maltoside (DDM) for 30 min, followed by sonication (6×10 s pulse with 10 s chill on ice) and centrifugation at 13000× g for 30 min. Cell lysates were then incubated with Ni-NTA agarose beads (Qiagen) for 120 min at 4°C. Ni-NTA beads were pelleted at 1000× g for 1 min; the beads were pipetted into columns and washed three times with 50 mM NaH2PO4 buffer (pH 8.0) containing 300 mM NaCl and 20 mM imidazole. Recombinant NAPE-1 and NAPE-2 were eluted from the Ni-NTA beads with 50 mM NaH2PO4 buffer (pH 8.0) containing 300 mM NaCl and 250 mM imidazole. Purified proteins were analyzed by SDS-PAGE (NuPAGE 4–12% Bis Tris gel) and their concentrations were determined using the Pierce 660 nm protein assay kit (Thermo Fisher) and immediately used for activity measurements.

Enzyme assays

The phospholipase-D activities of purified NAPE-1 and NAPE-2 were assayed in 200 µL Tris buffer (100 mM, pH 7.6) containing 0.5 mM DDM and 1 mM CaCl2 with N-arachidonoyl PE or N-palmitoyl PE as substrate [5]. Known amounts of the substrate were dried and re-suspended in the buffer mixture followed by addition of 1 µg of purified protein. The reactions were carried out for 4 hours at 20°C, and terminated by extraction twice with 400 µL hexane. Lipid extracts were dried down, derivatized with BSTFA and analyzed by GC-MS as described previously [17]. AEA-d4 and PEA-d4 were used as a standard.

C. elegans maintenance and strains

C. elegans strains were maintained as previously described [18]. Bristol N2 (wild-type), daf-2(e1368) III, fat-1(ok2323) IV, fat-4(ok958) IV and fat-3(wa22) IV were obtained from the Caenorhabditis elegans Genetics Center (University of Minnesota, MN). faah-1(tm5011) IV, nape-1(tm2860) IV and nape-2(tm6254) IV were obtained from Dr Shohei Mitani at the National Bioresource Project at Tokyo Women's Medical University School of Medicine and each strain was backcrossed 5 times to wild type prior to analysis.

Generation of transgenic lines

Translational C-terminal GFP or mCherry fusions were generated essentially as described by Hobert [19]. To generate the pnape-1::nape-1::mCherry construct, nape-1 coding sequence was amplified with 2 kb of the promoter region and fused to an mCherry::unc-54 3′UTR fragment. For generation of pnape-2::nape-2::gfp, nape-2 coding sequence and approximately 1.7 kb of the promoter region was fused to a gfp::unc-54 3′UTR fragment of pPD95.75 (gift from Andrew Fire). The resulting constructs were microinjected into the gonad of young adult worms and transgenic animals were identified in the next generation by their expression of the co-injection marker unc-25::mrfp. At least four independent transgenic lines were analyzed. A representative line was chosen for integration using trimethylpsoralen/UV mutagenesis. The resulting integrated lines, containing the transgenes jluIs7(nape-1::mCherry unc-25::mrfp) and jluIs2(nape-2::GFP unc-25::mrfp), were outcrossed to wild type five times before analysis and are referred to as nape-1(OE) and nape-2(OE), respectively. To visualize co-localization of nape-1::mCherry and nape-2::gfp without interference from the co-injection marker a non-integrated transgenic line was generated by co-injecting pnape-1::nape-1::mCherry and pnape-2::nape-2::gfp without the unc-25::mrfp marker (resulting line jluEx71(nape-1::mCherry nape-2::gfp).

Genetic crosses

A strain over-expressing both nape-1 and nape-2 was generated by crossing jluIs7 with jluIs2. The nape single over-expressers were also crossed into the faah-1(tm5011), daf-2(e1368), fat-1(ok2323), fat-4(ok958) and fat-3(wa22) mutant backgrounds by standard methods. A daf-2(e1368); fat-4(ok958) double mutant was also generated and crossed with fat-4(ok958); jluIs7 and fat-4(ok958); jluIs2 to generate daf-2(e1368); fat-4(ok958); jluIs7 and daf-2(e1368); fat-4(ok958); jluIs2, respectively. Mutants containing daf-2(e1368) were verified by direct sequencing of the daf-2 mutation, while faah-1(tm5011), nape-1(tm3860), nape-2(tm6254), fat-1(ok2323) and fat-4(ok958) genotypes were confirmed by PCR. Double mutants with fat-3(wa22) were confirmed by phenotype.

Confocal imaging

Fluorescence images were acquired at 40× magnification using an Olympus FluoView 1000 laser scanning confocal microscope such that fluorescence was within the limits of under- and over-exposure. Image quantification was carried out using Image J software. Briefly, individual Z-stack images were combined into one image and normalized for brightness and contrast. Fluorescence intensity measurements were determined by subtracting background fluorescence from the region of interest (ROI). The size of the ROI was kept the same for all samples within a replicate.

Growth assays

Worms were conditioned at each temperature for a minimum of two generations prior to examining growth, except for studies in the fat mutant backgrounds, in which worms were maintained at 20°C and not conditioned at the assay temperature. Eggs from a one hour synchronous lay were collected and incubated at 15°C, 20°C or 25°C for a time period sufficient for the wild type controls to reach adulthood (2 days at 25°C, 3 days at 20°C and 5 days at 15°C). Animals were scored for their developmental stage after this time period. Analysis was performed using Prism 4 software (Graphpad Software, Inc.). The raw data for the growth experiments are presented in Table S1.

Dauer assays

Dauer assays were performed as previously described [20], [21]. In brief, for dauer entry assays, eggs from a synchronous lay were transferred to assay plates and incubated at 25°C. After 3 days, the plates were scored for the presence of dauer and non-dauer larvae based on morphology. For the dauer recovery assays, eggs from a synchronous lay were transferred to assay plates and incubated at 25°C. After 3 days, dauers were selected by treatment with 1% sodium dodecyl sulfate (SDS) for 15 minutes, transferred to a fresh plate and incubated at 20°C for 24 h. Recovery was scored by counting dauer and non-dauer animals after treatment with 1% SDS.

Lifespan analysis

Lifespan analysis was performed as previously described [17]. Worms were maintained at 20°C and eggs from a synchronous lay were transferred to the appropriate temperature. For daf-2 lifespans at 25°C, all strains were raised at 20°C and shifted to 25°C as first day adults to avoid dauer arrest. On the first day of adulthood, animals were transferred to plates containing 2 µg/mL 5-fluorodeoxyuridine (FUdR), to inhibit progeny production, with the exception of lifespans carried out at 15°C where no FUdR was used. Each condition was assayed in duplicate with 50 worms per plate. Worms were transferred to new plates every two days and transferred to plates without FUdR at day 8. Survival analysis was performed using Prism software (Graphpad Software, Inc.); Kaplan-Meier survival curves were plotted for each lifespan assay and compared using the Log-rank test. Animals that either crawled off the plate, experienced internal hatching or exhibited vulval protrusion were treated as censored objects in the survival analysis.

Mass culture of worms for GC-MS

Mass cultures were maintained at 20°C. Starved L1s from eggs prepared by sodium hypochlorite treatment were used to seed 10 cm NGM plates spotted with 2 mL concentrated E. coli OP50. Adult worms were harvested from plates seeded with 20000–25000 starved L1s. For growth at 15°C and 25°C starved L1s from 20°C cultures were shifted to the appropriate temperature and harvested as adults (2 days at 25°C and 5 days at 15°C). Harvested worms were washed 3 times in S-basal, snap frozen in liquid nitrogen and stored at −80°C. A 20 µL aliquot was used to determine the total protein in the sample, using the bicinchoninic acid assay (BCA Protein Assay Kit, Thermo Scientific) with modifications for use with nematodes [22], [23].

Measurement of NAE levels by GC-MS

For NAE quantification, lipid extraction and solid phase fractionation was carried out as previously described [17]. GC-MS analysis was carried out as previously described [17] with the following alterations. Samples were analyzed in triplicate, corresponding to at least 333 mg worms per run. Following derivatization with BSTFA for 60 min, samples were dried down under nitrogen to a volume of 1 µL. GC-MS analysis was performed using an Agilent 7890A GC and 240-ion trap MS system operating in splitless mode with a VF-5 ms capillary column (30 m×0.25 mm i.d., 5% phenyl-95% methyl polysiloxine, 0.25 µm film thickness; Varian, Inc., Walnut Creek, CA). GC conditions: Injector 280°C. Initial column temperature was 150°C for 1 min and then ramped at 20°C per min to 300°C followed by a 5°C ramp to 325°C and then held for 10 min. MS conditions: Analytes were chemically ionized using acetonitrile vapor and data was collected using the MRM mode in Agilent MS Workstation software version 7.0.0. Precursor ions were isolated using an isolation window of 3. MS/MS fragmentation was performed in the ion trap using an excitation storage level of 164.0, excitation amplitude of 80, and non-resonant collision energy for all analytes. Palmitoleoyl ethanolamine (POEA), linoleoyl ethanolamine (LOEA) and eicosapentaenoyl ethanolamine (EPEA) were quantified with reference to the PEA-d4 internal standard and expressed as the amount of NAE per mg of protein.

Results

There are two C. elegans genes with homology to the mammalian NAE biosynthetic enzyme NAPE-PLD, nape-1 (Y37E11AR.4) and nape-2 (Y37E11AR.3) that are adjacent to each other in the genome. nape-1 and nape-2 are predicted to express transcripts of 1348 bp and 3077 bp respectively, sharing 73% identity at the DNA sequence level, and producing similar sized protein products that have 84% identity and 92% similarity (Figure 1A). Both NAPE-1 and NAPE-2 retain all of the highly conserved residues in the NAPE-PLD signature sequence HX(E/H)XD(C/R/S/H)X50–70HX15–30(C/S/D)X30–70H [7], [24].

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Figure 1. C.elegans NAPE-1 and NAPE-2 have NAPE-PLD activity and are expressed in overlapping and distinct tissues.

(A) Alignment of C. elegans NAPE-1 and NAPE-2 amino acid sequences with human, mouse and rat NAPE-PLD. Both NAPE-1 and NAPE-2 contain all the key catalytic residues (highlighted in black boxes) characteristic of NAPE-PLD in mammals. Recombinant NAPE-1 (B) and NAPE-2 (C) are capable of generating arachidonoyl ethanolamine (AEA) from N-arachidonoyl phosphatidylethanolamine (N-arachidonoyl PE) in vitro. (D) Confocal microscopy image showing expression and co-localization of pnape-1::nape-1::mCherry and pnape-2::nape-2::gfp in the nervous system and pharynx.

https://doi.org/10.1371/journal.pone.0113007.g001

To confirm that the C. elegans NAPE-PLD orthologs are capable of synthesizing NAEs, we expressed recombinant His-tagged NAPE-1 and NAPE-2 in E. coli C41(DE3) cells from the pET28a expression vector and examined their ability to generate NAEs in vitro. Expression of the recombinant proteins was confirmed by SDS PAGE and the identities of purified NAPE-1 and NAPE-2 confirmed by LC/MS (Figure S1). Freshly purified NAPE-1 and NAPE-2 were capable of liberating arachidonoyl ethanolamine (AEA) from its precursor molecule N-arachidonoyl PE (Figure 1B and C), and no such AEA release was observed in controls lacking any protein (Figure S1). Similar results were obtained with another NAPE-PLD substrate, N-palmitoyl PE, which yielded palmitoyl ethanolamine (Figure S1). These data indicate that both C. elegans NAPE-1 and NAPE-2 are capable of generating NAEs and confirms that they are functional orthologs of NAPE-PLD.

To examine where nape-1 and nape-2 are expressed in vivo, we generated a transgenic strain that expressed each of the enzymes, under the control of their endogenous promoters, fused to either mCherry (nape-1) or GFP (nape-2) fluorescent tags. Both enzymes are expressed predominantly in the pharynx (Figure 1D), but nape-2 is also highly expressed in the dorsal and ventral nerve cords, as well as being strongly expressed in the vulval muscles of hermaphrodites (Figure S2). nape-1 is also expressed in these areas, but at very low levels, and is only seen in the cell bodies of the dorsal and ventral nerve cords (Figure S2).

We had previously observed that over-expression of the NAE degrading enzyme faah-1 resulted in slowed growth and increased lifespan [17]. We therefore predicted that loss of nape-1 or nape-2 might lead to a similar phenotype. The nape-1 deletion mutant has a 483 bp in frame deletion that spans exons 2 and 3 and results in a predicted 214 aa peptide that lacks part of the NAPE-PLD signature sequence. The nape-2 deletion mutant has a 476 bp deletion/32 bp insertion that removes exon 1 and part of exon 2. After backcrossing to wild type, neither the nape-1 nor nape-2 deletion had any effect on growth or lifespan at any temperature (Figure 2 and S3).

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Figure 2. Deletion of nape-1 or nape-2 has no effect on growth or lifespan.

There was no effect of the nape-1(tm3860) or nape-2(tm6254) deletions on growth at (A) 15°C, (B) 20°C or (C) 25°C compared with the wild type N2 strain. Data are presented as mean+s.d for 6 (15°C), 3(20°C) and 5 (25°C) biological replicates. (D–F) Lifespan was not significantly affected by nape-1 or nape-2 deletion at any temperature. Data shown are representative of three biological replicates. Summary data, statistical analysis and additional lifespan data are presented in Figure S3.

https://doi.org/10.1371/journal.pone.0113007.g002

Since there was no strong phenotype in either the nape-1 or nape-2 deletion mutants, we examined the effect of over-expression of each enzyme under the control of their respective native promoters. Given the level of homology between the two isoforms we hypothesized that over-expression of both nape-1 and nape-2 together would result in a stronger phenotype than either over-expresser alone. When grown at the standard temperature of 20°C, there was a subtle, low penetrance growth delay in the nape-2(OE) strain that was maintained, but not strengthened in the nape-1(OE); nape-2(OE) animals (Figure 3B). Interestingly, the growth phenotypes of the nape over-expressing strains diverged when grown at 15°C and 25°C. At 15°C, nape-1(OE) showed mild growth delay similar to that seen at 20°C, but in nape-2(OE) at 15°C there was a significant fraction of animals that arrested at the first larval stage (L1) of development, with only 37% of animals reaching larval stage 4 (L4) after 5 days, compared with 99% in wild type (Figure 3A). Interestingly, at this temperature, the phenotype of the nape-1(OE); nape-2(OE) animals more closely resembled the nape-1(OE) strain, suggesting that the effects of nape-2(OE) were mitigated by the presence of the nape-1 transgene (Figure 3A). In contrast, at 25°C nape-2(OE) animals showed a mild growth defect, but in nape-1(OE) animals there was a pronounced growth delay with only 21% of animals reaching the L4 stage after 2 days, compared with 99% in wild type (Figure 3C). At this temperature, animals over-expressing both nape-1 and nape-2 showed a phenotype similar to that of nape-1 alone (Figure 3C).

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Figure 3. Over-expression of nape-1 and nape-2 affect development and lifespan in a temperature dependent manner.

(A) At 15°C, nape-2(OE) worms showed significant growth delay that was characterized by L1 arrest, while the phenotype of nape-1(OE) worms was not different from controls and nape-1(OE); nape-2(OE) animals showed an intermediate phenotype (mean+sd, n = 9 except nape-1(OE); nape-2(OE) where n = 4, ANOVA p<0.0001, pairwise comparisons vs N2 **p<0.01, ***p<0.001). (B) At 20°C, nape-2(OE) and nape-1(OE); nape-2(OE) showed mild growth delay compared with N2 (n = 4, ANOVA p<0.01, pairwise comparison vs N2 **p<0.01). (C) At 25°C, nape-1(OE) worms showed the strongest growth delay, which was mirrored by the nape-1(OE); nape-2(OE) strain (n = 9 except nape-1(OE); nape-2(OE) where n = 4, ANOVA p<0.0001, pairwise comparisons vs N2 *p<0.05, ***p<0.001). (D) At 15°C, nape-2(OE) showed a small but significant increase in lifespan (p<0.01) while nape-1(OE) were not different compared with wild type. (E) At 20°C, there was no significant effect of nape-1(OE) or nape-2(OE) on lifespan. (F) At 25°C, nape-1(OE) showed a significant reduction in lifespan (p<0.0001), but there was no effect of nape-2(OE). Data shown are representative of replicate experiments. Summary data, statistical analysis and additional lifespan data are presented in Figures S4, S5, S6.

https://doi.org/10.1371/journal.pone.0113007.g003

In terms of lifespan, there was no strong effect of nape-2 over-expression at any temperature, but at 15°C lifespan was slightly increased in 3/5 trials (Figure 3D–F, Figures S4, S5, S6). At 15°C and 20°C, lifespan of nape-1 over-expressers was not different from wild type, but at 25°C nape-1(OE) lifespan was significantly reduced compared with N2 in 4/6 trials (Figure 3D–F, Figures S4, S5, S6). The phenotype of worms over-expressing both nape-1 and nape-2 tracked with nape-2 at 15°C and with nape-1 at 25°C (Figures S4, S5, S6). Taken together, the growth and lifespan data suggest that despite strong sequence homology and shared ability to generate NAEs in vitro, NAPE-1 and NAPE-2 may function differently in vivo in response to temperature.

We have previously shown that global over-expression of faah-1 reduced NAE levels and that RNAi of faah-1 increased NAE levels [17]. We therefore hypothesized that loss of faah-1 activity would exacerbate the growth phenotypes conferred by nape over-expression by further elevating NAE levels. The faah-1(tm5011) mutant contains a 515 bp deletion that removes the second exon of the gene and is likely a null. Consistent with our hypothesis, we found that the faah-1 deletion enhanced the growth delay of nape-1 over-expressers at both 15°C and 25°C (Figure 4A). Surprisingly, loss of faah-1 in the nape-2(OE) strain completely rescued the L1 arrest observed at both temperatures, implying that loss of faah-1 mitigates the effects of nape-2 over-expression (Figure 4B).

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Figure 4. Loss of faah-1 enhances nape-1(OE) phenotypes but suppresses nape-2(OE).

(A) faah-1(tm5011) enhances the growth delay of nape-1 over-expressers at both 15°C and 25°C (mean+sd, N2 and nape-1(OE) n = 9 and others n = 5 replicates, ANOVA p<0.0001 at each temperature, *** p<0.001 and * p<0.05 for indicated pairwise comparisons). (B) faah-1(tm5011) suppresses the L1 arrest of nape-2 over-expressers at both 15°C and 25°C (mean+sd, N2 and nape-2(OE) n = 9 and others n = 5 replicates, ANOVA p<0.0001 at each temperature, *** p<0.0001, ** p<0.01 and *p<0.05 for indicated pairwise comparisons). (C) NAE levels in nape-1(OE) and faah-1(tm5011); nape-1(OE) grown at 15°C were not significantly elevated (mean+sd, faah-1(tm5011) n = 12, nape-1(OE) and faah-1(tm5011); nape-1(OE) n = 7 replicates, one sample test for deviation from 100% - *p<0.05). (D) NAE levels in nape-1(OE) and faah-1(tm5011); nape-1(OE) grown at 25°C showed a significant linear trend towards increased levels (mean+sd, faah-1(tm5011) n = 9, nape-1(OE) n = 8 and faah-1(tm5011); nape-1(OE) n = 6 replicates, one sample test for deviation from 100% - *p<0.05). ***p<0.0001 and *p<0.05 for the linear trend are indicated above the solid lines. (E) At 15°C NAE levels in nape-2(OE), but not faah-1(tm5011); nape-2(OE), were elevated (mean+sd, faah-1(tm5011) n = 12, nape-2(OE) and faah-1(tm5011); nape-2(OE) n = 7 replicates, one sample test for deviation from 100% - *p<0.05). (F) NAE levels in nape-2(OE) and faah-1(tm5011); nape-2(OE) grown at 25°C were not different from N2 or from each other (mean+sd, faah-1(tm5011) n = 9, nape-2(OE) n = 6 and faah-1(tm5011); nape-2(OE) n = 5 replicates). (G) There was no change in NAPE-1::mCherry fluorescence intensity in the faah-1(tm5011) deletion background at 15°C and only a minor decrease at 25°C (*p<0.05). Data are from n = 10 worms for each strain and are representative of three independent replicates. (H) There was a significant reduction in NAPE-2::GFP expression in the faah-1(tm5011) deletion background at both 15°C and 25°C (***p<0.0001). Data are from n = 10 worms for each strain and are representative of three independent replicates at 15°C, and 2 independent replicates at 25°C.

https://doi.org/10.1371/journal.pone.0113007.g004

Given that NAPE-1 and NAPE-2 are capable of generating NAEs in vitro we hypothesized that NAE levels would be altered in the nape over-expressers. At 15°C, NAE levels in nape-1(OE) were not significantly elevated compared with control animals (Figure 4C). However, at 25°C EPEA in nape-1(OE) and POEA and EPEA in faah-1(tm5011); nape-1(OE) were higher than N2, and there was also a significant linear trend towards higher levels of each NAE levels across the strains (Figure 4D). These data are consistent with the appearance of stronger growth and lifespan phenotypes at 25°C in nape-1 over-expressers and suggest that nape-1(OE) has a greater effect on NAE levels at 25°C compared to 15°C.

At 15°C NAE levels in nape-2(OE) were significantly higher than N2 but there was not a statistically significant increase at 25°C. This is consistent with stronger nape-2(OE) growth phenotypes at 15°C. NAE levels in faah-1(tm5011); nape-2(OE) did not show any statistically significant differences at either temperature, but there was a tendency for the higher levels in nape-2(OE) to be reduced by the presence of the faah-1 deletion (Figure 4E & F). This is consistent with the observation that the faah-1 deletion rescued the growth phenotype of nape-2(OE) animals (Figure 4B) and suggests that loss of faah-1 reduces nape-2 expression or activity. To provide a molecular basis for this effect, we examined the level of the fluorescently tagged NAPE-PLDs in the faah-1 deletion background. There was no significant difference in nape-1::mCherry levels at 15°C and only a minor reduction at 25°C in faah-1(tm5011); nape-1(OE) compared with nape-1(OE), suggesting that the increased levels of NAEs in the faah-1(tm5011); nape-1(OE) background was not due to an increase in nape-1 protein (Figure 4G). In contrast, we found that there was a significant reduction in nape-2::gfp levels in the faah-1 deletion background at both 15°C and 25°C (Figure 4H), suggesting that the reduction of NAEs in the faah-1(tm5011); nape-2(OE) strain could be due to reduced nape-2 protein expression.

The NAE measurements indicated a tendency toward elevated EPEA levels in the nape-1 over-expressing strain at 25°C, where this strain showed the strongest growth delay. In our previous study we had observed that exogenous treatment of wild type animals with EPEA did not have any deleterious effect on growth and fertility [17], suggesting that other NAEs may be responsible for the growth delay. To examine growth in the absence of C20 NAEs such as EPEA, we crossed the nape over-expressing strains with mutants that are unable to synthesize the fatty acid precursors for these long-chain NAEs. fat-1, fat-4 and fat-3 encode fatty acid desaturases and mutations in these genes lead to specific fatty acid defects [25]. Loss of fat-1 results in the absence of eicosapentaenoic acid, the precursor for EPEA, and a corresponding increase in arachidonic acid, the precursor for AEA. Mutation of fat-4 leads to a failure to synthesize both arachidonic and eicosapentaenoic acid, but other C20 fatty acids are still present. Finally, loss of fat-3 generates an animal devoid of C20 polyunsaturated fatty acids. Loss of either fat-4 or fat-3, but not fat-1, resulted in growth delay in wild type and nape over-expressers at 15°C (Figure 5A). However, at 20°C, although there was no effect of either of the fat mutations on growth in non-transgenic animals, loss of fat-4 or fat-3 delayed growth in nape-1(OE), and loss of fat-4 significantly delayed growth in nape-2(OE) animals (Figure 5B). At 25°C, the delayed growth of nape-1(OE) animals was further exacerbated by each fat mutant, while only fat-4 and fat-3 further affected nape-2(OE) animals (Figure 5C). Taken together, these data suggest that the presence of C20 fatty acids, and by inference C20 NAEs, mitigates the deleterious effects of nape over-expression on growth and implies that it is NAEs other than EPEA that are causing the growth delay.

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Figure 5. The absence of C20 fatty acids enhances the growth defects in nape over-expressers.

(A) At 15°C, mutations in the fatty acid desaturases fat-4 and fat-3, but not fat-1, confer developmental delay in all strains (No transgene - ANOVA p<0.001, pairwise comparisons N2 vs fat-1 p = n.s, vs fat-4 p<0.05 and vs fat-3 p<0.001; nape-1(OE) – ANOVA p<0.0001, pairwise comparisons N2 vs fat-1 p = n.s, vs fat-4 p<0.001 and vs fat-3 p<0.0001; nape-2(OE) – ANOVA p<0.0001, pairwise comparisons N2 vs fat-1 p = n.s, vs fat-4 p<0.0001 and vs fat-3 p<0.0001). (B) At 20°C, mutations in the fatty acid desaturases have no effect in non-transgenic animals (ANOVA p = n.s.). However, growth of nape-1(OE) animals is influenced by fat-4 and fat-3 (ANOVA p<0.0001, pairwise comparisons N2 vs fat-1 p = n.s, vs fat-4 p<0.0001 and vs fat-3 p<0.0001), whereas nape-2(OE) animals are adversely affected by fat-4 only (ANOVA p<0.05, pairwise comparisons N2 vs fat-1 p = n.s, vs fat-4 p<0.05 and vs fat-3 p = n.s.). (C) At 25°C, there is a mild effect of the fat-3 mutation on growth of non-transgenic animals (ANOVA p<0.05, pairwise comparisons N2 vs fat-1 p = n.s., vs fat-4 p = n.s. and vs fat-3 p<0.05). At this temperature, the growth defect of nape-1(OE) animals is further enhanced by all fat mutants (ANOVA p<0.0001; pairwise comparisons nape-1(OE) vs fat-1 p<0.05, vs fat-4 p<0.001 and vs fat-3 p<0.05). Growth of nape-2(OE) animals was affected only by fat-4 and fat-3, but not fat-1 (ANOVA p<0.0001; pairwise comparisons nape-2(OE) vs fat-1 p = n.s., vs fat-4 p<0.001 and vs fat-3 p<0.001). Data are presented as mean+sd for 4 replicates at 15°C and 20°C and 5 replicates at 25°C. The milder growth phenotype of the nape-2(OE) animals at 15°C in these experiments is due to the fact that these animals had not been conditioned at the lower temperature prior to growth studies.

https://doi.org/10.1371/journal.pone.0113007.g005

In our previous study we had also observed that EPEA treatment suppressed dauer entry and reduced lifespan in daf-2 insulin receptor mutants [17]. We therefore examined the effect of nape over-expression on dauer formation and lifespan in daf-2 mutants. There was no effect of either nape-1(OE) or nape-2(OE) on daf-2(e1368) lifespan at 20°C, but at 25°C nape-1(OE) resulted in a significant reduction in daf-2 lifespan (Figure 6A & B, Figures S5 & S7). There was also a small suppression of dauer formation in both the nape over-expressers at the restrictive temperature of 25°C (Figure 6C), as well as an increase in the number of animals that recovered from dauer after 24 h at the permissive temperature of 20°C (Figure 6D). These data suggest that an increase in the endogenous level of EPEA enhances dauer recovery. To test this further, we examined dauer recovery in a daf-2; fat-4 mutant background and found a significant reduction in basal dauer recovery in the daf-2; fat-4 double mutant compared with daf-2 alone (Figure 6D). Loss of fat-4 in the daf-2; nape-1(OE) and daf-2; nape-2(OE) backgrounds also reduced dauer recovery (Figure 6D), supporting the idea that endogenous EPEA levels influence dauer recovery.

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Figure 6. nape over-expression modulates lifespan and dauer formation in daf-2 mutants.

(A) nape-1 or nape-2 over-expression has no effect on lifespan of daf-2(e1368) mutants at 20°C. (B) nape-1(OE), but not nape-2(OE), suppresses daf-2(e1368) lifespan at 25°C (p<0.0001). (C) nape-1(OE) and nape-2(OE) have a small but significant suppressive effect on dauer formation in daf-2(e1368) at 25°C (mean+sd, n = 4 replicates). (D) nape-1(OE) and nape-2(OE) enhances dauer recovery in daf-2(e1368). Loss of the fatty acid desaturase fat-4, which eliminates EPEA and AEA, leads to reduced dauer recovery in daf-2(e1368), daf-2(e1368); nape-1(OE) and daf-2(e1368); nape-2(OE) (mean+sd, n = 9 trials from 3 biological replicates ANOVA p<0.0001, pairwise comparisons *p<0.05, **p<0.01, ***p<0.001).

https://doi.org/10.1371/journal.pone.0113007.g006

Discussion

We have previously determined that C. elegans has a functional NAE system, through the identification of multiple NAE molecules and the observation that the activity of the NAE degradation enzyme, FAAH, was conserved [17]. In this study, we have focused on characterizing the worm orthologs of the NAE biosynthetic enzyme NAPE-PLD.

In mammals, and other species, there is a single NAPE-PLD that generates NAEs from the phospholipid N-acyl phosphatidyl ethanolamine (NAPE). Comparative genomics had previously identified Y37E11AR.4 (nape-1) as a C. elegans ortholog of NAPE-PLD [9] and we had identified another candidate, (Y37E11AR.3, nape-2). Given their sequence similarity, and their adjacent location in the genome, it is highly likely that nape-1 and nape-2 arose from a gene duplication event, a phenomenon that is common in C. elegans [26], [27]. Here we show that the recombinant proteins, expressed and purified from bacteria, retain their NAPE-PLD activity and when over-expressed in C. elegans nape-1 and nape-2 modulate NAE levels, consistent with their proposed function. NAPE-2 appeared to be more effective in the in vitro assays, but whether this is due to differences in the protein preparations or a true reflection of substrate preference remains to be determined.

Translational fusions of nape-1 and nape-2, driven by their respective endogenous promoters, indicated that expression was primarily in the pharynx, which is consistent with the expression of a nape-1 transcriptional fusion and the expression of faah-1 [17]. However, nape-2 appeared to be more broadly expressed, with fluorescence also observed in the nerve ring, the dorsal and ventral nerve cords, and the reproductive system. The overlap in their expression pattern was restricted to small distinct areas within the pharynx suggesting that nape-1 and nape-2 may have undergone functional divergence, which is common in duplicated genes in C. elegans [26]. However, the fact that each enzyme was able to generate both a short chain, saturated NAE (PEA) and a long-chain, polyunsaturated NAE (AEA) in vitro, suggests that spatial and temporal differences in expression pattern or substrate availability may drive the difference in function more than differences in substrate specificity.

In our previous work, reduced NAE levels, arising from over-expression of faah-1, were associated with delayed growth [17], but in the current study, single deletion mutants of nape-1 and nape-2 did not affect growth at any temperature. It is possible that a deletion of both nape-1 and nape-2 would have a stronger phenotype than either single mutant, but we were unable to generate such a mutant because of the close proximity of the two genes in the genome. However, it is also possible that there are alternate pathways generating NAEs in C. elegans that are independent of NAPE-PLD, as has been observed in mammals [7], [28][32], which could minimize the effect of nape deletion.

Given that neither nape-1 nor nape-2 deletion conferred an obvious phenotype, we focused on phenotypes associated with nape-1 or nape-2 over-expression. Surprisingly, nape-1 over-expression conferred a generalized delay in development, while nape-2 over-expression resulted in a partially penetrant L1 arrest phenotype. Perhaps more surprising was the observation that growth and lifespan phenotypes varied with temperature, with nape-1 over-expressers more severely affected at 25°C and nape-2 over-expressers more adversely affected at 15°C. There did not appear to be any major changes in transgene expression at each temperature that could explain the phenotypic differences (Figure S8). In many other systems NAPE-PLD and FAAH appear to have broad specificities suggesting that the exact composition of the NAE profile is a consequence of other factors such as substrate availability and/or composition [1], [33].

The NAE system is thought to be an on-demand system, in that the activity of a given NAE is determined by the balance between its synthesis and degradation [1]. Based on this, we reasoned that loss of function of the degrading enzyme encoded by faah-1 would enhance the phenotypes associated with NAPE-PLD over-expression. We found this to be the case for the faah-1(tm5011); nape-1(OE) strain, but in contrast, we found that loss of faah-1 suppressed the L1 arrest phenotype of the nape-2(OE) strain. Further characterization of this strain indicated that there was a reduction in nape-2::gfp expression from the transgene in the presence of the faah-1 deletion. One explanation for this phenomenon is that there is a negative feedback loop in which high NAE levels arising from faah-1 deletion down-regulate nape-2 expression, to maintain NAE levels within a physiological range. Such a mechanism has been proposed both in mice and Arabidopsis [34], [35]. Alternatively, there may be as yet unidentified NAEs that are produced independently of NAPE-2, and that are metabolized by FAAH-1, that act to suppress nape-2 expression. Interestingly, such a feedback loop does not appear to operate with nape-1, since loss of faah-1 exacerbated the nape-1(OE) growth phenotype. One possibility is that nape-1 activity is coupled to one of the other faah orthologs that are found in the C. elegans genome that have yet to be characterized. Taken together, these data point toward differences in the regulation of the two NAPE-PLD homologs, and further support the functional divergence between the two.

The magnitude of the increase in NAEs in the nape over-expressing strains was relatively small. This could be related to the fact that NAEs are likely to signal over short distances, and thus small changes in the local NAE environment may have a large phenotypic effect and not be reflected in systemic or global NAE levels. Moreover, measurement of NAEs in each over-expression strain did not identify specific changes that could explain differences in the nape-1(OE) and nape-2(OE) phenotypes. However, a disadvantage of the GC-MS method we use to measure NAE is that we only detect what we look for and thus there may be other, as yet undescribed NAE species that are altered in response to nape over-expression which could potentially be detected with an unbiased analytical approach [35], [36]. Another possibility, that we were not able to test in the current study, is that the phospholipid substrate for NAPE-PLD, NAPE, itself has a specific biological function. Thus, over-expressing the nape enzymes could result in changes in NAPE availability in specific tissues which affect developmental and aging phenotypes. In this respect, a specific biological function for NAPE has been proposed in other species [35], [37].

To date we have not identified a biological role for the C16 and C18 NAEs found in worms. However, the exacerbation of the growth defects in nape over-expressers lacking C20 fatty acids and NAEs suggests that one or more of the shorter chain NAEs could be responsible for the deleterious effects on growth. In contrast, we had previously observed that EPEA suppressed entry into the dauer larval stage, and reduced adult lifespan [17]. The observation that nape-1(OE), but not nape-2(OE), suppressed lifespan in both wild type, as well as daf-2 mutants is consistent with the observed elevation in EPEA levels in this strain at 25°C. A new finding in the current study was that recovery from the dauer stage was augmented in daf-2 mutants carrying the nape transgenes. This phenotype appears to be, at least in part, related to EPEA since we were able to show that loss of EPEA, via inactivation of the fatty acid desaturase fat-4, resulted in reduced recovery from the dauer larval stage in both the daf-2 single mutant and in daf-2 animals carrying either nape-1(OE) or nape-2(OE) transgenes. Taken together these data suggest that EPEA may have a role in signaling resumption of reproductive growth following arrest in the dauer larval stage.

In summary, we have shown that the C. elegans orthologs of NAPE-PLD, NAPE-1 and NAPE-2, are able to synthesize NAEs in vitro, in a manner that is consistent with a conservation of biochemical function, and further reinforces the nematode as a genetic model system for studying NAE physiology. While the response to environmental temperature in poikilotherms such as C. elegans has conventionally been viewed as a passive thermodynamic response, recent studies suggest that different genetic programs modulate the response to high and low temperatures, particularly with respect to aging [38], [39]. The differing effects of nape-1 and nape-2 over-expression in response to temperature could suggest a role for NAE signaling in these genetically encoded thermal response programs.

Supporting Information

Figure S1.

Recombinant NAPE-1 and NAPE-2 generate N-acylethanolamines from N-acyl phosphatidylethanolamine substrates in vitro. His-tagged NAPE-1 and NAPE-2 were expressed in E. coli C41(DE3) cells and the identity of the purified protein was confirmed by LC-MS. Two samples were analyzed for each protein and peptide coverage for a representative sample is shown for NAPE-1 (A) and NAPE-2 (B). (C) NAPE-1 and NAPE-2 generate AEA from N-arachidonoyl PE, and no AEA is detected from control reactions that lack protein. Both NAPE-1 (D) and NAPE-2 (E) also liberated PEA in vitro from N-palmitoyl PE substrate.

https://doi.org/10.1371/journal.pone.0113007.s001

(DOCX)

Figure S2.

nape-1::mCherry and nape-2::gfp expression in other tissues. Confocal microscopy images showing pnape-1::nape-1::mCherry (A&D) and pnape-2::nape-2::gfp (B&E) and co-localization (C&F). A–C show representative confocal images indicating that nape-2 but not nape-1 is expressed in the dorsal nerve cord. D–F show representative confocal images indicate that nape-2 is expressed in the vulva.

https://doi.org/10.1371/journal.pone.0113007.s002

(DOCX)

Figure S3.

Summary of lifespan experiments with nape-1 and nape-2 deletion strains.

https://doi.org/10.1371/journal.pone.0113007.s003

(DOCX)

Figure S4.

Summary of lifespan experiments with nape over-expressing strains at 15°C.

https://doi.org/10.1371/journal.pone.0113007.s004

(DOCX)

Figure S5.

Summary of lifespan experiments with nape over-expressing strains at 20°C.

https://doi.org/10.1371/journal.pone.0113007.s005

(DOCX)

Figure S6.

Summary of lifespan experiments with nape over-expressing strains at 25°C.

https://doi.org/10.1371/journal.pone.0113007.s006

(DOCX)

Figure S7.

Summary of lifespan experiments with nape over-expressers in the daf-2 background at 25°C.

https://doi.org/10.1371/journal.pone.0113007.s007

(DOCX)

Figure S8.

nape-1::mCherry and nape-2::gfp expression is not affected by changes in growth temperature. Confocal images of nape-1(OE) and nape-2(OE) worms grown at (A) 15°C and (B) 25°C. The dashed lines in the nape-1(OE) images indicate the unc-25::mrfp co-injection marker.

https://doi.org/10.1371/journal.pone.0113007.s008

(DOCX)

Acknowledgments

Some strains were provided by the CGC, which is funded by NIH Office of Research Infrastructure Programs (P40 OD010440).

Author Contributions

Conceived and designed the experiments: NH MAL PRR IVO MSG. Performed the experiments: NH MAL TKK IVO MSG. Analyzed the data: NH MAL MSG. Wrote the paper: NH MAL PRR MSG.

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