Ascaroside Pheromones: Chemical Biology and Pleiotropic Neuronal Functions

Abstract

In 1982, the first biological evidence of a nematode pheromone was reported by the Riddle group, who showed that a partially purified C. elegans extract could trigger dauer formation in L1/L2 larvae [12]. [...]unless otherwise stated, our discussion will be limited to ascr pheromones and their potential neuronal functions. 2.2. [...]the Sternberg group showed that the difference of ascaroside blends between many nematode species was observed with respect to variance of ascr pheromone composition [39]. [...]the source of the ascarylose moiety was an interesting question.

1. What Are Pheromones?

Pheromones are neuronal signaling molecules synthesized by various organisms and then excreted into the environment, where they typically stimulate individuals of the same species to react to environmental changes (e.g., temperature shifts, biological stimuli, or nutritional changes) [1,2]. It is thought that most organisms, from prokaryotes to higher animals such as humans, can produce and use pheromones for communication between conspecific individuals. In most cases, pheromones trigger neuronal events that are linked to various behavioral responses. The outcomes of such neuronal stimulation are the modulation of developmental and/or physiological programs that can support adaptation to new environments [3]. For example, approximately 1500 insect pheromones have been identified since bombykol was discovered in 1959 [4]. These pheromones mediate common behaviors such as courtship rituals, mating, aggregation, dispersal (e.g., spacing or epideictic pheromones), alarm, recruitment (e.g., trailing pheromones), and maturation [2,4]. In mammals, pheromones are used for marking territories, and for signaling mating and feeding preparedness [5,6].

In humans, there have been numerous reports of putative pheromones; however, their existence has not been experimentally confirmed. For example, a putative human pheromone was proposed to be excreted from the apocrine gland in the male underarm, although its functions have not been characterized [7,8]. Unlike other mammals, humans lack a functional vomeronasal organ (VNO), which processes pheromonal signals in mice and other vertebrates [8,9,10]. The absence of this key VNO function makes the discovery of human pheromones even more challenging.

The Caenorhabditis elegans dauer pheromone, which is part of an important chemical language throughout this nematode’s lifespan, has long been known. In 1975, Cassada and Russell first reported the existence of dauer larvae, an alternative developmental stage that prolongs survival under environmental conditions that do not support growth [11]. The observation of dauer larvae might have provoked the search for dauer pheromones. In 1982, the first biological evidence of a nematode pheromone was reported by the Riddle group, who showed that a partially purified C. elegans extract could trigger dauer formation in L1/L2 larvae [12]. Indeed, this pioneering work inspired worm biologists to continue to search for pure dauer pheromones.

2. Structural Diversity of Ascaroside (ascr) Pheromones 2.1. Daumone, the First Chemically Characterized Ascr Pheromone

In 2005, the Paik group isolated and chemically characterized the first C. elegans pheromone, which they named dauer pheromone, or daumone (now often referred to as ascr#1) [13]. Via an activity-guided purification procedure using 300 L of cultured worms, they isolated pure daumone, which has the molecular formula C₁₃H₂₄O₆ and an M_r of 276 (Figure 1). Determination of the stereochemical structure of purified daumone, [(2)-(6R)-(3,5-dihydroxy-6-methyltetrahydro-pyran-2-yloxy) heptanoic acid], revealed that it contains one ascarylose (a 3,6-dideoxy sugar also known as rhamnose) linked to the C7 of a methylated short-chain fatty acid (mSCFA) (Figure 1).

They also demonstrated that natural and chemically synthesized daumone could equally induce dauer formation in the wild-type C. elegans laboratory strain (N2) and in Caenorhabditis briggsae. The discovery of daumone, which is indeed a bona fide signaling molecule, not only settled a long-time dispute as to whether the C. elegans pheromone acted as a signal or a crowd cue [14], it also opened a new avenue for investigating the chemical biology of ascr pheromones on molecular and system-wide scales. As additional dauer pheromone derivatives (collectively called ascarosides) were identified, daumone was later renamed ascaroside #1 (ascr#1) as per Edison’s suggestion [15], which was based on the presence of an ascarylose sugar moiety linked to an mSCFA. In this review, we use “ascr pheromones” rather than ascarosides to distinguish between the pheromones and non-pheromonal ascr derivatives or metabolites, consistent with the terminology used for steroid hormones (i.e., steroids vs steroid hormones). This distinction is important, given that more than 200 ascaroside-like compounds with unknown functions have now been identified via metabolomic methods [16,17].

Historically, non-pheromonal ascarosides were first identified among the neutral lipids of parasitic nematodes such as Ascaris lumbricoides and Parascaris equorum [18,19]. These compounds typically consist of a glycone moiety (one or two ascarylose units, i.e., a 3,6-dideoxy sugar) and an aglycone moiety, a very long chain fatty acid (VLCFA) that contains greater than or equal to 25 carbon atoms [20]. They were mainly recovered from the eggs and reproductive tract tissue of female A. lumbricoides nematodes, and they were shown to confer the eggs with chemical resistance against external toxic insults [21]. Therefore, unless otherwise stated, our discussion will be limited to ascr pheromones and their potential neuronal functions.

2.2. Identification of Diverse Ascr Pheromones in Nematodes

In the 15 years since the discovery of the first ascr pheromone, several groups have intensely investigated their chemical biology. For instance, the Clardy group energized the pheromone research community by identifying two additional ascr pheromones (i.e., ascr#2 and 3) in cultured worms [22]. Ascr#2 and 3 contain essentially the same structural backbone as ascr#1 (C7-SCFA) but differ in the number of carbons in the mSCFA moiety linked to the 3,6-dideoxy ascarylose sugar (ascr#2: C6-mSCFA with a methyl ketone, ascr#3: α-β unsaturated C9-mSCFA) (Figure 2). To distinguish the ascr pheromone families in this article, we classify them into two groups: the simple ascr pheromones, which contain only ascarylose and mSCFA, and the modular ascr pheromones, which contain modified ascarylose. Other simple and modular ascr pheromones have now been identified and characterized [16,23,24,25,26,27]. In particular, the Schroeder group detected small amounts of several ascarosides (i.e., ascr#6.1, 6.2, 7, and 8) among the metabolites of the wild-type N2 strain by comparing its two-dimensional nuclear magnetic resonance spectrum with that of the ascaroside biosynthesis-defective daf-22(m130) strain [25]. These ascr pheromones contain an unsaturated seven-carbon mSCFA linked to a p-aminobenzoate subunit (i.e., ascr#8) or β-glucose (i.e., glas#10) [25] (Figure 2).

The indole carboxy (IC) ascarosides (icas, e.g., icas#1, 3, 7, 9, and 10) contain a unique indole-3-carbonyl unit attached to the 4′-position of ascarylose [24,27] (Figure 2). Profiling of worm extracts via MS/MS fragmentation and GC-EIMS led to the identification of approximately 200 additional ascr derivatives [16,17]. Notably, structural variations were found in the carbon chain lengths of the mSCFA moiety (e.g., ascr#18, 21, 22, and 25). More examples are the presence of hydroxybenzoyl (hbas#3) or 2-methyl-2-butenoyl moieties (mbas#3) attached to the 4′-position of the ascarylose, ω-linkages at the terminal carbons of the mSCFA moieties, and 2′-hydroxylation of the mSCFA (Figure 2).

Most functionally characterized ascr pheromones are ω-1 linked, i.e., a methyl group is attached to the C1 position at the link between the mSCFA and the ascarylose; however, ω-linked ascr pheromones lacking this linkage have also been reported [16,23] (Figure 2). The structural diversity in the mSCFA is likely generated via the multi-cycled peroxisomal β-oxidation that occurs during ascaroside biosynthesis, although other mechanisms are possible [16,28,29,30,31,32,33,34,35,36]. Some structural derivatives of ascr pheromones contain other functional groups (e.g., a methyl group, amino acid precursor, glucose, or benzoyl group) linked to the 2′- or 4′-position of the ascarylose moiety or to the 1′-position of the mSCFA moiety, generating a collection of highly diverse ascaroside structures (Figure 2). It is worth noting that ascr pheromone-like derivatives have also been identified in other nematode genera [37,38,39,40,41,42]. Moreover, the Sternberg group showed that the difference of ascaroside blends between many nematode species was observed with respect to variance of ascr pheromone composition [39]. As most known ascr derivatives share a common structural backbone but differ in their mSCFA moieties or ascarylose modifications (Figure 2), determining their individual functions will be a daunting task.

3. Ascr Pheromone Biosynthesis and Metabolic Regulation 3.1. Ascr Pheromone Biosynthesis

Initially, it was proposed that the ascr pheromone precursors are produced via two distinct reaction pathways, peroxisomal β-oxidation for the SCFA moiety and de novo biosynthesis for the ascarylose moiety (both the simple and modified forms). To produce mature, active ascr pheromone, the SCFA and ascarylose moieties would then be conjugated by UDP (uridine diphosphate)-glucuronosyl transferase (UGT) [29]; however, an alternative pathway has now been proposed. In this alternative pathway, a VLCFA-conjugated ascarylose is first produced and then subsequently subjected to peroxisomal β-oxidation to produce active ascr pheromone [43,44]. This proposal was supported by genetic screens and metabolomic experiments. In maoc-1, dhs-28, and daf-22 mutant strains, most of the ascarosides with fatty acid chain lengths of less than nine carbons are not synthesized, whereas non-pheromonal FA-conjugated ascarylose (e.g., VLCFA-, VLCFA-CoA-, and LCFA (long-chain fatty acid linked ascarylose)) accumulates in the worm body [16,17,29,30,43].

Naturally, the source of the ascarylose moiety was an interesting question. The Paik group previously demonstrated that the ascarylose was not derived from the Escherichia coli consumed by the worms, but rather that it was de novo synthesized [29]. Sorting out this issue was necessary because ascarylose (a glycoconjugate of ascaroside) is found in the lipopolysaccharide (LPS) of Gram-negative bacteria, and it represents a unique class of sugars with a 3,6-dideoxy sugar structure [45]. In bacteria such as Yersinia pseudotuberculosis, ascarylose is produced via a continuous chain of five enzymatic reactions in which CDP-D-glucose is produced from glucose-1-phosphate [46,47,48]. However, in the course of studying egg shell formation, a gene responsible for ascarylose biosynthesis was found in C. elegans [49], supporting the earlier argument in favor of de novo ascarylose biosynthesis [29]. However, additional work is needed to elucidate the detailed mechanism of this step in C. elegans.

UGT might be an ideal candidate for catalyzing the conjugation of ascarylose to VLCFAs, as occurs during detoxification reactions in mammals [50,51]. The basis of this prediction is that during detoxification, UGT transfers the monosaccharide glucuronic acid to lipophilic metabolites (e.g., steroids and bile acids) and xenobiotics (e.g., environmental toxins) to render them water-soluble for release [52,53,54]. However, it remains unknown in C. elegans whether an enzyme similar to UGT might catalyze the linkage of fatty acids to ascarylose or cooperate with other enzymes to specifically synthesize ascarosides. For instance, the enzyme encoded by dgtr-1, which is involved in egg shell formation, is also thought to be required for ascaroside synthesis because of its homology to the DGAT2 family of acyl-CoA:diacylglycerol acyltransferases, which catalyze the addition of fatty acyl-CoA to diacylglycerol to form triacylglycerol [49].

During the biosynthesis of modular ascarosides (e.g., icas, mbas, hbas, and osas), several organic moieties (e.g., amino acid metabolites) are attached to the 4′-position of ascarylose. Using deuterium-labeled tryptophan and axenic in vitro culturing, the Schroeder group found that the indole carbon atom of icas is derived from l-tryptophan, while the 4-hydroxybenzoyl group of hbas is derived from l-tyrosine or l-phenylalanine. Furthermore, the tigloyl group of mbas and the octopamine succinyl group of osas are derived from l-isoleucine and l-tyrosine, respectively [16,55]. It has also been suggested that lysosomal ACS-7, an acyl-CoA synthase, catalyzes the linkage of indole-3-carboxy (icas) or N-succinyl octopamine groups to ascr [32]. However, the Butcher group showed that ACS-7 appears to transport icas to the peroxisomes during the biosynthesis of the short-chain ascaroside icas [36]. This dispute on the function and cellular location of ACS-7 remains to be resolved. Based on the findings discussed above, a working model for the biosynthesis of both simple ascr (no attached organic moieties) and modular ascr (various attached organic moieties) in C. elegans can be proposed (Figure 3). In this scheme, cytochrome P450 generates (ω-1) or ω-oxygenated VLCFA or LCFA precursors that are then linked to ascarylose to form FA-linked ascarosides (e.g., LCFA). The FA-linked ascarosides then enter the peroxisomal β-oxidation pathway to produce active mSCFA ascr pheromones [16,49].

Peroxisomal β-oxidation is a central metabolic pathway in animals that supplies SCFA components for energy production in mitochondria as well as the main carbon chain precursors for ascr pheromones. The presence of peroxisomes in the intestine and hypodermis of C. elegans and the target signals of their peroxisomal proteins have been revealed [56,57]. This topic has been covered in detail by recent publications, and the field is still evolving; therefore, this discussion focuses on important developments related to the production of the mSCFA moieties used in ascr pheromones, as the mSCFAs are a key driver of the structural and functional diversity of ascr pheromones. Research on the ascr biosynthetic pathway has progressed well since the discovery of the nematode acyl-CoA oxidases (ACOX-1 or ACOX-1.1) [30]. ACOXs catalyze the first reaction of peroxisomal β-oxidation by producing enoyl-CoA from acyl-CoA, and they contribute to maintaining the ascr pheromone pool synthesized in response to sudden environmental shifts [30]. Some ascr pheromones (i.e., ascr#2, and 3) are not synthesized by the acox-1 (ok2257) mutant strain [30], whereas the synthesis of others (ascr#1, 9, 10, oscr#9, and 10) is elevated [16]. These observations suggest that the acox-1 gene produces multiple ACOX isoforms, which were later found to have different substrate specificities [33,34,35]. The Butcher group used CRISPR/Cas9 genome editing to elegantly produce various mutant derivatives of the ACOX isoforms and found that the different ACOX isoforms can form various homo- and heterodimers with distinct substrate preferences that produce different ascr pheromones. For example, the ACOX-1.1/ACOX-1.4 heterodimer produces ascr#1 while the ACOX-1.1/ACOX-1.3 heterodimer produces ascr#2 [35]. This mechanism for the biosynthesis of such diverse ascr pheromones by the ACOX isoforms is supported by the observation that ACOXs might act on (ω-1)- and ω-oxygenated VLCAs prior to their cyclic stepwise breakdown during peroxisomal β-oxidation. Furthermore, this finding also confirms an earlier report that the ACOXs help to define the ascr pheromone population produced by C. elegans [30]. For the second and third reactions of the peroxisomal β-oxidation pathway, MAOC-1 hydrates enoyl-CoA to produce hydroxyacyl-CoA and DHS-28 dehydrogenates hydroxyacyl-CoA to produce 3-ketoacyl-CoA [16,28,29]. Finally, mature mSCFA-containing ascr pheromones are produced via the thiolase activity of DAF-22, a homolog of human SCPx.

3.2. Transcriptional Regulation of Ascr Pheromone Biosynthesis by Environmental Stressors

Although sequence of the biosynthesis of ascr pheromones is known well, it remains unknown how these enzymes are transcriptionally regulated by environmental changes (e.g., temperature increases, nutrition deprivation). To address this question, it was essential to quantify the levels of the approximately ~200 ascr derivatives currently known in C. elegans, and to accurately measure the changes in the levels of the ascr pheromones under various physiological states via a standard quantification method [58,59,60]. The Paik group developed the “PheroQu” method, a multiple reaction monitoring (MRM)-based ascr pheromone quantification method that uses ultra-performance liquid chromatography coupled to mass spectrometry (MS) with only 20 worms. This method enables accurate quantification of the levels of various ascrs in the worm body and in the medium during larval development [59]. With this method, it was found that the biosynthesis of several ascr pheromones (ascr#1-3) is robustly influenced by developmental stage, growth condition, and environmental stress (e.g., heat) throughout the life cycle [59].

Upon an increase in ambient temperature, the levels of ascr pheromones increase up to two-fold [30]. It was later found that heat-shock factor 1 (HSF-1) regulates the transcription of ascaroside synthesis genes (e.g., acox-1, dhs-28, and daf-22) in response to external temperature. This finding was supported by chromatin immunoprecipitation assays and increased production of chemically detectable ascarosides (e.g., ascr#1 and 3) [31]. Based on this observation, it appears that C. elegans requires transcriptional regulation to ensure that a sufficient ascr supply is available upon encountering sudden environmental changes or stress signals, such as poor nutrition or high population density, to prepare for dauer entry. Related to this concept, the Butcher group recently reported that poor nutrition and high temperature can lead to the transformation of one type of ascr (e.g., aggregation-inducing medium-chain icas) into another type (e.g., dauer-inducing short-chain icas), providing evidence of flexibility in the structure and function of ascr pheromones in response to environmental stress [33,36]. Thus, via combinatorial usage of the products of the acox gene family, C. elegans has multiple options for adapting to new environments without expending metabolic energy and resources [36].

4. Pleiotropic Neuronal Functions of Ascr Pheromones 4.1. Roles of Ascr Pheromones in Development and Aging

The ascr pheromones influence a variety of functions in the chemosensory neurons that control development, aging, and behaviors in conspecific individuals. Depending on their concentration in the media, they also trigger other important behaviors (e.g., dauer-induction, lifespan extension, mating attraction, repulsion, aggregation, and foraging) that are essential for survival under stressful conditions [26,36,61,62]. Perhaps the best-known function of ascr pheromones is their ability to induce dauer entry, which is a unique system for prolonged survival in C. elegans. Reports from several groups showed that there are robust changes in the expression levels of various genes in dauer larvae and dauer entry and exit [63,64,65,66]. These findings indicate that ascr pheromones exert their biological functions via some less-characterized signaling pathways involved in neuronal transmission [13,15,26].

By taking advantage of the availability of ascr pheromones, the Paik group characterized the real-time metabolic molecular landscape during dauer formation. These data revealed the metabolic changes underlying the worm’s adaptation during the developmental shift to diapause. They measured the genome-wide gene expression changes via DNA microarrays that cover 22,250 unique genes. Their results suggested the presence of a unique adaptive metabolic control mechanism that requires both stage-specific expression of specific genes as well as tight regulation of different modes of fuel metabolite utilization to sustain the energy balance for prolonged survival under adverse conditions [63]. A comprehensive web-based dauer metabolic database for C. elegans is available (www.DauerDB.org) for use by the research community and might be broadly useful as a molecular atlas for related nematodes. In addition, using the chemically available pure ascr pheromones, the Lee group routinely produced C. elegans dauer larvae and explored that IL2 neurons mediate a phoretic behavior of dauer larvae, called nictation [67]. Furthermore, the same group also characterized nictation as a means of dispersal and survival strategy under harsh conditions through interspecific interaction of C. elegans dauer larvae [68].

The clarification of the molecular pathways involved in dauer induction raised questions about the presence of ascr pheromone receptors, which should mediate pheromone sensing to elicit dauer entry. At least three putative pheromone receptors that directly trigger the relevant signaling pathways have been identified in several nematode species. The first ascr pheromone receptor was reported by the Sengupta group, who discovered that the G protein-coupled receptors (GPCRs) SRBC-64 and SRBC-66 are expressed in ASK neurons where they are required for pheromone-induced dauer formation [69]. However, srbc-64(tm1946) and srbc-66(tm2943) mutant worms failed to form dauer larvae in response to ascr#1–3 but entered the dauer stage normally in response to ascr#5 [69]. The decrease in the calcium level in the ASK neurons in response to ascr pheromone observed in adult wild-type worms was not detected in the srbc-64(tm1946) and srbc-66(tm2943) strains. These mutants did not exhibit long-term responses to pheromones, indicating that other pheromone receptors function via competing signaling cascades depending on the developmental stage [70]. The Bargmann group reported that two other GPCRs, SRG-36 and SRG-37 (which belong to the serpentine receptor class), might act as ascr#5-specific ascr pheromone receptors that relay the same dauer entry signals in the ASI neurons [71]. They took advantage of two C. elegans strains (LSJ2 and CC1) that had been propagated for long periods of time in liquid axenic media that, unlike the wild-type N2 strain, did not form dauer larvae in response to ascr pheromones (ascr#1, 2, 3, and 5). Quantitative trait locus (QTL) mapping and whole-genome sequencing revealed single-nucleotide polymorphisms in srg-36 and srg-37 in LSJ2 and CC1, respectively, that specifically prevented the response to ascr#5. In C. briggsae, another nematode species, the receptor encoded by an srg gene paralogous to srg-36 and srg-37 responds to ascr#5 [71]. These results indicate that remodeling of the chemoreceptor repertoire in nematodes allows adaptation to the external environment and that changes in paralogous genes may have common effects across species. In 2012, the Riddle group found that DAF-37 and DAF-38 (also GPCRs) function as a heterodimer to respond to ascr pheromones [72]. DAF-37 responds specifically to ascr#2, and its expression in ASI neurons regulates ascr#2-mediated dauer formation, whereas its expression in ASK neurons regulates adult behavior. DAF-38, on the other hand, plays a cooperative role in sensing ascr#2, 3 and 5 [72]. Other candidate molecules involved in pheromone-induced dauer formation were identified using a forward genetic screen; however, they seem to function in pheromone signaling rather than as pheromone receptors [73,74]. The findings that different pheromone-responsive receptors are expressed in different neurons suggest that additional receptor molecules in other neurons might remain to be identified.

The Scheroder group recently found that ascr#2, a ligand of the DAF-37 ascr receptor, mediates an approximately 20% lifespan extension in a sirtuin-dependent manner [75]. This finding revolutionized our thinking on how dauer formation is involved in lifespan extension in C. elegans. This new concept, known as ascr-mediated increases of lifespan (AMILS), represents a new paradigm for chemosensation-based non-dauer lifespan extension as it is independent of DAF-16-governed insulin signaling and DAF-12. Given the availability of other ascr pheromones, it would be interesting to investigate whether AMILS is specific to ascr#2 or whether it exists in other nematode genera or can be regulated by other ascr pheromones.

4.2. Neuronal Effects of Ascr Pheromones on Nematode Social Behaviors

As described above, ascr pheromones have a wide spectrum neuronal functions that not only mediate dauer entry, but also influence adult behaviors and phenotypes, including lifespan extension. For example, very low concentrations (fM–pM) of ascr pheromones attract males, whereas higher concentrations (nM–μM) promote dauer entry [26] (Figure 4). Ascr#3, in particular, seems to act as a strong male-attracting pheromone, and various concentrations of ascr#2–4 appear to exhibit strong synergistic roles in amphid single-ciliated sensory neurons (ADF/ASK) and cephalic companion neurons (CEM) [26,76,77]. Ascr#8 is also an important male-attracting pheromone at both low and high concentrations [25,76]. These findings clearly confirm that ascr pheromones have neuronal functions that trigger diverse behaviors to ensure prolonged survival in response to environmental changes.

Interestingly, although ascr#1–3 induce dauer entry of L1 worms at higher concentrations (nM–μM), similar concentrations act as chemorepellents after the L1 stage that stimulate hermaphrodite repulsion [26,62,77,78,79,80]. These observations suggest that these pheromones act in a concentration-dependent and stage-specific manner. These repulsive responses appear to be transmitted via the GPA-3-DAF-16/FOXO signaling pathway in sensory neurons, and they affect long-term memory via glutamate signaling regulated by DAF-16 [78]. Note that this behavior is distinct from male attraction behavior because the genetic sex modulates the sensitivity of the ADF neurons to ascr pheromones [77]. The ascr#3-dependent avoidance behavior is stimulated by ascr#3 sensing in the ADL neurons followed by signal propagation to the interneurons, which then regulate the magnitude of the behavioral changes stimulated by pheromone contact in relation to feeding state or early larval development [79,80]. Furthermore, mbas#3 (an ascaroside linked to a tigloyl group) and osas#9 (an ascaroside linked to a succinyl octopamine group) also have repulsive effects similar to those of ascr#3 and icas#3 [55,81].

At low concentrations (< 10 nM), ascr#2, 3, and 5 can attract hermaphrodites only in specific social strains or strains lacking NPR-1 (e.g., the npr-1(ad609) mutant), an important regulator of aggregation behavior [62]. At low concentrations, some IC group-containing ascr pheromones (e.g., icas#1, icas#3, and icas#9) induce aggregation in solitary N2 hermaphrodites as well as in naturally isolated social strains (e.g., CB4856 and RC301), while they induce male attraction at higher concentrations [27]. These responses require the ASK sensory neurons and downstream AIA neurons, but not the RMG neuron required for attraction in npr-1(ad609) mutants as previously reported. Like the icas pheromones, ascr#1, 2, 3, and 5 can act as chemorepellents or aggregation-inducing pheromones, suggesting that their activity is determined by their environmental concentrations. At low concentrations, they induce attraction, whereas at higher concentrations they induce repulsion. One group reported that this behavioral change also depends on the oxygen concentration [82]. In this study, the authors found that RMG neurons control the oxygen concentration via the URX neurons, resulting in switching between attraction signals in ASK neurons and repulsion signals in ADL neurons. The discovery of the icas#9 receptors, encoded by srx-43 and srx-44, via QTL mapping and whole-genome sequencing [61,83] revealed that SRX-43 is expressed in ASI neurons, whereas SRX-44 is expressed in ASJ and ADL neurons, and that roaming behavior is determined by the site of their expression [83].

In several asexual species, the rate of sexual reproduction increases in stressful environments, functioning as a survival strategy to generate genetic variation via recombination during outcrossing [84,85,86,87,88,89,90,91,92]. In C. elegans, ascr pheromones induce male mating or aggregation behavior in the early survival state. For example, two naturally occurring strains (CB4856 and JU440) exhibit increased male frequency during the dauer stage that is not observed in the N2 laboratory strain N2. This effect is due to an increase in the male mating rate and increased male survival during the dauer period [93]. The male attraction behavior in response to ascr pheromones is thought to induce an increase in male frequency in dauer-inducing environments [15]; thus, it is likely that larger male populations are beneficial for survival in unfavorable external environments. One study reported that the hermaphrodite reproductive rates of some other naturally isolated strains are regulated by secreted pheromones [94]. In fact, ascr#3 and 10 are secreted at different rates by males and hermaphrodites [95]. A combination of ascr pheromones secreted by males has been reported to not only affect the hermaphrodite reproductive system, but also to increase heat stress resistance [96]. This male-secreted pheromone also has a male-killing effect, thereby regulating the population size of the species [97]. In sum, the functions and structure of some ascr pheormones are listed in Table 1.

The concentrations of the ascr pheromones produced by worms and their main functional changes in response to external environmental conditions are outlined in Figure 4. Under favorable conditions, the ascr pheromone concentrations are too low to exert any effects, perhaps due to other environmental factors. However, ascr pheromone synthesis gradually increases as worms encounter unfavorable stress conditions (e.g., high temperature, food limitation, and high population density) [30,59]. It has been hypothesized that ascr pheromones stimulate male mating or aggregation at relatively low concentrations under normal growth conditions, while under stressful conditions that trigger increased ascr pheromone production (and thus higher concentrations), worms may exhibit a repulsive response to ascr pheromone and enter the dauer state. However, the structural basis for the functional differences between ascr pheromones has not yet been clarified.

5. Implications of Ascr Pheromone Metabolism in Neuroprotection 5.1. Implications of Ascr Pheromone Biosynthesis Gene Deficiencies in Neuronal Disorders

Several ascr pheromone biosynthesis defects have been identified in mutant worms deficient for peroxisomal β-oxidation enzymes [16,28,29,30,31,32,33,34,35,36,98]. The physiological consequences of impaired DAF-22-dependent peroxisomal β-oxidation of VLCFAs or fatty acyl-CoAs involved in the production of various aglycone units (mSCFAs with less than nine carbon atoms) required for pheromone biosynthesis indicate that peroxisomal β-oxidation of VLCFAs is an essential detoxification process for clearing harmful peroxisomal fatty acids to maintain cellular homoeostasis. This function indicates that ascr pheromones not only regulate stress avoidance, they also maintain cellular homeostasis via the production of excretable FA-ascarylose conjugates (ascarosides) [29]. Here we examine the pleiotropic neuronal functions of ascr pheromones from two different angles, ascr metabolic deficiency and chemotactic responses.

In mammals, it is well known that peroxisomal malfunctions induce developmental defects and neurodevelopmental diseases. These diseases include Zellweger syndrome (ZS) and X-linked adrenoleukodystrophy (X-ALD), which involve severe neurological problems that often lead to death in infants and young children [99,100,101,102,103,104]. In humans, a single defect in an enzyme involved in peroxisomal fatty acid β-oxidation leads to ZS, which involves abnormal symptoms such as neonatal hypotonia, craniofacial dysmorphia, seizures, and developmental delay [100,103,104,105]. Mechanistically, it was suggested that the defect in peroxisomal fatty acid β-oxidation results in the accumulation of VLCFAs in the form of triacylglycerols, which are harmful to animals [29,105]. Furthermore, decreased docosahexaenoic acid (DHA; C22:6 (n-3)) levels, plasmalogen depletion, and abnormal neurons myelination (e.g., degenerative loss of myelin (demyelination) or abnormally formed myelin (dysmyelination)) have been suggested to underlie the neuropathologies associated with peroxisomal disorders [106]. In C. elegans, ascaroside biosynthesis appears encompass two important physiological roles that affect the worm’s quality of life: (1) a social function in which pheromone production affects the behavior and physiology of other individuals, and (2) protection of metabolic homeostasis via the removal of toxic VLCFAs in peroxisomes (Figure 5) [29].

In addition to neurodevelopmental defects, deficiencies in peroxisomal fatty acid β-oxidation seem to be related to other pathologies. In C. elegans, animals deficient in peroxisomal fatty acid β-oxidation, such as the dhs-28(tm2581) and daf-22(ok693) mutant strains, exhibit short lifespans and developmental delays, and are more susceptible to environmental stresses, limiting the worm’s survival under harsh conditions [29,107]. In particular, it has recently been suggested that peroxisomal fatty acid β-oxidation has distinct functions in neuronal cells for maintaining normal development and nervous system function [101,106,107]. More interestingly, it was revealed that neuronal peroxisomal fatty acid β-oxidation has an important cell-autonomous function to regulate neuroendocrine signaling activities [107]. The C. elegans SCPx gene daf-22 is expressed in a subset of chemosensory neurons, i.e., the ASK neurons, where its activity is required for exogenous pheromone-induced dauer entry [107]. A deficiency in neuronal peroxisomal fatty acid β-oxidation activates the lipid-induced endoplasmic reticulum (ER) stress response, which then increases the expression of insulin-like peptides in neurons and abnormally enhances insulin/IGF-1 signaling activity to eventually interrupt dauer entry [107]. Meanwhile, ER stress-mediated dauer diapause is also regulated by other sensory neurons, such as the ASI neurons [108]. It has been suggested that the mutated DAF-28 peptide in the daf-28(sa191) mutant strain triggers ER stress and activation of the unfolded protein response (UPR) to induce constitutive dauer entry [108,109,110,111].

From these studies, it can be inferred that peroxisomal fatty acid β-oxidation is important for neuroprotection via the regulation of metabolic homeostasis (e.g., balance in fatty acid levels), myelination of neuronal cells, and the regulation of cellular signaling; these neuroprotective functions could influence aging, neurodevelopment, and stress resistance. Therefore, it is important to investigate the mechanisms underlying the roles of neuronal peroxisomal fatty acid β-oxidation in neuroprotection and aging in the future. It would also be worthwhile to elucidate the links between neuronal peroxisomal disorders and alterations in neuronal function and neurodevelopment (Figure 6).

5.2. Implications of Ascr Pheromone Signaling in Chemotactic Responses

Ascr pheromones induce a variety of behaviors [112]; however, these behaviors are controlled not only by the ascr pheromones but also by various other associated factors and environmental conditions. In general, food signals play important roles in determining behaviors and developmental choices in the presence of ascr pheromones in C. elegans. For example, calcium/calmodulin-dependent protein kinase I (CMK-1) regulates pheromone-mediated dauer entry in ASI/AWC neurons depending on the feeding state, although not directly via a pheromone-binding receptor [113]. Furthermore, gut-to-neuron signaling induced by feeding conditions affects TGF-β and insulin expression via target of papamycin complex 2 (TORC2), which leads to dauer entry or behavioral changes [114]. Repulsive behavior in response to feeding status is also induced by pheromone-mediated insulin signaling [80]. The combination of these two signals determines the choice between dauer entry or progression to the reproductive state via downstream regulation of DAF-12 and the associated let-7 microRNA family and hunchback-like-1 (HBL-1) [115]. Ascr pheromones are also involved in chemotactic behavior by regulating endogenous peptide signaling [116]. C. elegans exhibits chemotactic attraction toward odorants such as benzaldehyde; however, after prolonged exposure, the chemotactic behavior shifts to a dispersion behavior, and this shift is called olfactory adaptation or food-odor associative learning. The results of the study of Yamada et al. also suggest that NEP-2 (a homolog of the extracellular peptidase neprilysin) and SNET-1 (an NEP-2 suppressor peptide) regulate olfactory adaptation, and that an ascr pheromone that inhibits snet-1 expression is essential for olfactory adaptation [116].

Factors associated with ascr pheromones and their sensing have also been implicated in other physiological processes, such as aging [117,118,119,120]. This change in longevity is not only affected by ascr pheromones, but rather it is also influenced by a combination of other factors, including nutritional state and population density [75,121]. These pheromones act as a kind of warning signal by which C. elegans is informed in advance of ongoing changes in growth conditions (e.g., the ratio between food and pheromones). Triggering of this warning signal is also caused by other factors in addition to ascr pheromones. Typically, pathogen-induced avoidance in C. elegans has been studied in the context of the innate immune system [122,123]. Interestingly, it appears that the signaling in response to exposure to food bacteria and pathogenic bacteria and the downstream effects are similar, with the difference being the toxicity of the organisms to the worms [124]. Several factors simultaneously play important roles in ascr pheromone-mediated signaling and pathogen avoidance. First, NPR-1, which controls aggregation via ascr pheromones [62], also plays an important role in pathogen avoidance [125,126,127]. Like pheromones, pathogens are also recognized by sensory neurons [128,129]. Furthermore, the TGF-β ligand and insulin, which also play important roles in dauer entry, also appear to be involved in pathogen avoidance [130,131,132]. However, DAF-7, a TGF-β ligand, acts in the ASI/ASJ neurons during pathogenic avoidance but primarily in the ASI neurons during ascr pheromone sensing [130,131]. Finally, ER stress or UPR activation in sensory neurons can also be induced by pathogens [133,134,135,136]. It is plausible to predict that these physiological effects might involve the same factors to promote the survival of the nematode (Figure 6). Indeed, it has been reported that the use of ascr pheromone in a mammalian system has a therapeutic effect on hepatic inflammation [137,138]. Furthermore, ARTD, a combination of artemisinin and ascr pheromone, can also be used as an effective therapeutic agent in osteoclasts, where it shows a potent cancer inhibitory effect [139]. Thus, this relationship deserves further investigation in the future.

6. Conclusions and Future Directions

In this comprehensive review, we have highlighted some of the major achievements from the past 15 years since the discovery of the first ascr pheromone (ascr#1) [13]. The rapid developments in the ascr field have increased the depth of our knowledge with respect to biosynthetic pathways, ascr receptor-mediated neuronal signaling pathways, and potential neuro-physiological effects in animals. We would also like to add a few words on our views of the future of the ascr pheromone field. (i) Translational research: Given that their biosynthesis has been thoroughly investigated, now is a good time to construct a chemical biology map or database to catalog the structure-function relationships of the more than 200 members of the ascr family. Since some factors involved in ascr biosynthesis also have important neuronal functions in mammals, translation of what we know about nematode ascr pheromones into studies of metabolic diseases might be a promising future step. Some physiological functions of ascr pheromones are also involved in mammalian aging and disease; thus, these pheromones may have implications in human disease. It will also be interesting to unravel the roles of ascr#1 in disease model animals or mammalian cells [137,138,139]. (ii) Neuronal pheromone sensing and signaling: Ascr pheromone biosynthesis and their recognition and processing are equally interesting. Previous studies showed that pheromone sensing occurs in sensory neurons, and three receptors specific to some ascr pheromones have been found. However, as the number of newly discovered ascr pheromones increases, how they are sensed and responded to via potential common sensing and signaling pathways remains to be resolved. For example, several GPCRs act as ascr pheromone receptors; however, additional GPCRs have been found in other species [140,141]. Furthermore, several physiological effects induced by ascr pheromones are synergistic, i.e., single pheromones do not always act alone [23,26]. Thus, ascr pheromone sensing and signaling are likely complex and elaborately intertwined and untangling of these knots could provide important clues for understanding neuronal signaling in other species. Given that different ascr pheromones appear to mediate different behaviors across the nematode species depending on environmental conditions, it is reasonable to ask the question, what is the lowest common denominator that underlies the diverse biological functions of ascr pheromones? Fully addressing this question will require additional research on the chemical biology of pheromones in the future. (iii) Neuronal ascr signaling and behavior: Ascr pheromones were originally found while searching for the factors that influence dauer entry, and they have since been reported to be involved in various behaviors in addition to dauer entry. Interestingly, the effects associated with ascr pheromones are almost exclusively influenced by external environmental cues, many of which involve stress (e.g., poor nutrition, overcrowding, and heat). Therefore, it will be interesting to clarify the biological links between ascr function and stress responses as well as neuroprotection (i.e., the innate immune response, see Section 5.2.). (iv) Creation of pheromics:In a literature survey of ascr pheromone publications, we noticed many interdisciplinary pheromone research projects and a boom in omics technologies. Examples include, but are not limited to, molecular genetics, chemical biology, metabolomics, proteomics, and genomics. At this juncture, it could be beneficial to create the field of “pheromics” (pheromone omics) as a new subset of integrated disciplinary research area within chemical ecology with the goal of establishing and supporting a community of researchers involved in the systematic study of the pheromones of living organisms.

Name	Chemical Structure	Discovered Receptors	Functions	References
ascr#1		SRBC-64 SRBC-66	Dauer inducing activity Repulsion activity	[13,69,78]
ascr#2		DAF-37 DAF-38 SRBC-64 SRBC-66	Dauer inducing activity Repulsion activity Male attraction activity Foraging activity	[22,26,61,62,69,72,78,82]
ascr#3		SRBC-64 SRBC-66	Dauer inducing activity Repulsion activity Male attraction activity Foraging activity	[22,26,61,62,69,76,77,78,79,80,82]
ascr#4		Unknown	Dauer inducing activity Male attraction activity	[26]
ascr#5		SRG-36 SRG-37	Dauer inducing activity Repulsion activity	[23,62,71,82]
ascr#6.1		Unknown	Dauer inducing activity	[25]
ascr#8		Unknown	Dauer inducing activity Male attraction activity Foraging activity	[25,61,76]
icas#3		Unknown	Male attraction activity Aggregation activity	[27]
icas#9		SRX-43SRX-44	Dauer inducing activity Male attraction activity Aggregation activity Foraging activity	[24,27,61,83]
hbas#3		Unknown	Hermaphrodite attraction activity	[16]
mbas#3		Unknown	Repulsion activity	[16,81]
osas#3		Unknown	Repulsion activity	[55]

* The ascr pheromones listed here were selected based on their identified functions, and citation frequencies.

Author Contributions

Conceptualization, Y.-K.P., H.-J.J., and J.Y.P.; Supervision, Y.-K.P.; Validation, Y.-K.P.; Visualization, H.-J.J., H.K. and J.Y.P.; Writing-original draft, H.-J.J., J.Y.P. and S.P.; Writing-review and editing, J.Y.P. and Y.-K.P.

Funding

This study was supported by a grant from the National Research Foundation of Korea (2017R1A2B3003200 to Y.-K.P.).

Conflicts of Interest

Authors declare no conflict of interest.

© 2019 by the authors. Licensee MDPI, Basel, Switzerland. This article is an open access article distributed under the terms and conditions of the Creative Commons Attribution (CC BY) license (http://creativecommons.org/licenses/by/4.0/).

References

1. Karlson, P.; Lüscher, M. 'Pheromones': A New Term for a Class of Biologically Active Substances. Nature 1959, 183, 55.

2. Wyatt, T.D. Pheromones. Curr. Biol. 2017, 27, R739-R743.

3. Brennan, P.A.; Zufall, F. Pheromonal communication in vertebrates. Nature 2006, 444, 308.

4. Tillman, J.A.; Seybold, S.J.; Jurenka, R.A.; Blomquist, G.J. Insect pheromones-an overview of biosynthesis and endocrine regulation. Insect Biochem. Mol. Biol. 1999, 29, 481-514.

5. Abel, E.L. Alarm substance emitted by rats in the forced-swim test is a low volatile pheromone. Physiol. Behav. 1991, 50, 723-727.

6. McGlone, J.J.; Anderson, D.L. Synthetic maternal pheromone stimulates feeding behavior and weight gain in weaned pigs. J. Anim. Sci. 2002, 80, 3179-3183.

7. Wyatt Tristram, D. The search for human pheromones: The lost decades and the necessity of returning to first principles. Proc. R. Soc. B Biol. Sci. 2015, 282, 20142994.

8. Wysocki, C.J.; Preti, G. Facts, fallacies, fears, and frustrations with human pheromones. Anat. Rec. A. Discov. Mol. Cell. Evol. Biol. 2004, 281A, 1201-1211.

9. McGann, J.P. Poor human olfaction is a 19th-century myth. Science 2017, 356, eaam7263.

10. Meredith, M. Human Vomeronasal Organ Function: A Critical Review of Best and Worst Cases. Chem. Senses 2001, 26, 433-445.

11. Cassada, R.C.; Russell, R.L. The dauerlarva, a post-embryonic developmental variant of the nematode Caenorhabditis elegans. Dev. Biol. 1975, 46, 326-342.

12. Golden, J.W.; Riddle, D.L. A pheromone influences larval development in the nematode Caenorhabditis elegans. Science 1982, 218, 578-580.

13. Jeong, P.-Y.; Jung, M.; Yim, Y.-H.; Kim, H.; Park, M.; Hong, E.; Lee, W.; Kim, Y.H.; Kim, K.; Paik, Y.-K. Chemical structure and biological activity of the Caenorhabditis elegans dauer-inducing pheromone. Nature 2005, 433, 541-545.

14. Viney, M.E.; Franks, N.R. Is dauer pheromone of Caenorhabditis elegans really a pheromone? Naturwissenschaften 2004, 91, 123-124.

15. Edison, A.S. Caenorhabditis elegans pheromones regulate multiple complex behaviors. Curr. Opin. Neurobiol. 2009, 19, 378-388.

16. von Reuss, S.H.; Bose, N.; Srinivasan, J.; Yim, J.J.; Judkins, J.C.; Sternberg, P.W.; Schroeder, F.C. Comparative Metabolomics Reveals Biogenesis of Ascarosides, a Modular Library of Small-Molecule Signals in C. elegans. J. Am. Chem. Soc. 2012, 134, 1817-1824.

17. von Reuss, S.H.; Dolke, F.; Dong, C. Ascaroside Profiling of Caenorhabditis elegans Using Gas Chromatography-Electron Ionization Mass Spectrometry. Anal. Chem. 2017, 89, 10570-10577.

18. Fauré-Frémiet, E. Le Cycle Erminatif Chez l'Ascaris Megalocephala; Masson: Issy les Moulineaux, France, 1913.

19. Flury, F. Zur Chemie und Toxikologie der Ascariden. Arch. Für Exp. Pathol. Pharmakol. 1912, 67, 275-392.

20. Fouquey, C.; Polonsky, J.; Lederer, E. Chemical structure of ascarylic alcohol isolated from Parascaris equorum. Bull. Soc. Chim. Biol. 1957, 39, 101-132.

21. Bartley, J.P.; Bennett, E.A.; Darben, P.A. Structure of the Ascarosides from Ascaris suum. J. Nat. Prod. 1996, 59, 921-926.

22. Butcher, R.A.; Fujita, M.; Schroeder, F.C.; Clardy, J. Small-molecule pheromones that control dauer development in Caenorhabditis elegans. Nat. Chem. Biol. 2007, 3, 420-422.

23. Butcher, R.A.; Ragains, J.R.; Kim, E.; Clardy, J. A potent dauer pheromone component in Caenorhabditis elegans that acts synergistically with other components. Proc. Natl. Acad. Sci. USA 2008, 105, 14288-14292.

24. Butcher, R.A.; Ragains, J.R.; Clardy, J. An Indole-Containing Dauer Pheromone Component with Unusual Dauer Inhibitory Activity at Higher Concentrations. Org. Lett. 2009, 11, 3100-3103.

25. Pungaliya, C.; Srinivasan, J.; Fox, B.W.; Malik, R.U.; Ludewig, A.H.; Sternberg, P.W.; Schroeder, F.C. A shortcut to identifying small molecule signals that regulate behavior and development in Caenorhabditis elegans. Proc. Natl. Acad. Sci. USA 2009, 106, 7708-7713.

26. Srinivasan, J.; Kaplan, F.; Ajredini, R.; Zachariah, C.; Alborn, H.T.; Teal, P.E.A.; Malik, R.U.; Edison, A.S.; Sternberg, P.W.; Schroeder, F.C. A blend of small molecules regulates both mating and development in Caenorhabditis elegans. Nature 2008, 454, 1115-1118.

27. Srinivasan, J.; von Reuss, S.H.; Bose, N.; Zaslaver, A.; Mahanti, P.; Ho, M.C.; O'Doherty, O.G.; Edison, A.S.; Sternberg, P.W.; Schroeder, F.C. A Modular Library of Small Molecule Signals Regulates Social Behaviors in Caenorhabditis elegans. PLOS Biol. 2012, 10, e1001237.

28. Butcher, R.A.; Ragains, J.R.; Li, W.; Ruvkun, G.; Clardy, J.; Mak, H.Y. Biosynthesis of the Caenorhabditis elegans dauer pheromone. Proc. Natl. Acad. Sci. USA 2009, 106, 1875-1879.

29. Joo, H.-J.; Yim, Y.-H.; Jeong, P.-Y.; Jin, Y.-X.; Lee, J.-E.; Kim, H.; Jeong, S.-K.; Chitwood, D.J.; Paik, Y.-K. Caenorhabditis elegans utilizes dauer pheromone biosynthesis to dispose of toxic peroxisomal fatty acids for cellular homoeostasis. Biochem. J. 2009, 422, 61-71.

30. Joo, H.-J.; Kim, K.-Y.; Yim, Y.-H.; Jin, Y.-X.; Kim, H.; Kim, M.-Y.; Paik, Y.-K. Contribution of the peroxisomal acox gene to the dynamic balance of daumone production in Caenorhabditis elegans. J. Biol. Chem. 2010, 285, 29319-29325.

31. Joo, H.-J.; Park, S.; Kim, K.-Y.; Kim, M.-Y.; Kim, H.; Park, D.; Paik, Y.-K. HSF-1 is involved in regulation of ascaroside pheromone biosynthesis by heat stress in Caenorhabditis elegans. Biochem. J. 2016, 473, 789-796.

32. Panda, O.; Akagi, A.E.; Artyukhin, A.B.; Judkins, J.C.; Le, H.H.; Mahanti, P.; Cohen, S.M.; Sternberg, P.W.; Schroeder, F.C. Biosynthesis of Modular Ascarosides in C. elegans. Angew. Chem. Int. Ed. 2017, 56, 4729-4733.

33. Zhang, X.; Feng, L.; Chinta, S.; Singh, P.; Wang, Y.; Nunnery, J.K.; Butcher, R.A. Acyl-CoA oxidase complexes control the chemical message produced by Caenorhabditis elegans. Proc. Natl. Acad. Sci. USA 2015, 112, 3955-3960.

34. Zhang, X.; Li, K.; Jones, R.A.; Bruner, S.D.; Butcher, R.A. Structural characterization of acyl-CoA oxidases reveals a direct link between pheromone biosynthesis and metabolic state in Caenorhabditis elegans. Proc. Natl. Acad. Sci. USA 2016, 113, 10055-10060.

35. Zhang, X.; Wang, Y.; Perez, D.H.; Jones Lipinski, R.A.; Butcher, R.A. Acyl-CoA Oxidases Fine-Tune the Production of Ascaroside Pheromones with Specific Side Chain Lengths. ACS Chem. Biol. 2018, 13, 1048-1056.

36. Zhou, Y.; Wang, Y.; Zhang, X.; Bhar, S.; Jones Lipinski, R.A.; Han, J.; Feng, L.; Butcher, R.A. Biosynthetic tailoring of existing ascaroside pheromones alters their biological function in C. elegans. eLife 2018, 7, e33286.

37. Bose, N.; Ogawa, A.; von Reuss, S.H.; Yim, J.J.; Ragsdale, E.J.; Sommer, R.J.; Schroeder, F.C. Complex Small-Molecule Architectures Regulate Phenotypic Plasticity in a Nematode. Angew. Chem. Int. Ed. 2012, 51, 12438-12443.

38. Bose, N.; Meyer, J.M.; Yim, J.J.; Mayer, M.G.; Markov, G.V.; Ogawa, A.; Schroeder, F.C.; Sommer, R.J. Natural Variation in Dauer Pheromone Production and Sensing Supports Intraspecific Competition in Nematodes. Curr. Biol. 2014, 24, 1536-1541.

39. Choe, A.; von Reuss, S.H.; Kogan, D.; Gasser, R.B.; Platzer, E.G.; Schroeder, F.C.; Sternberg, P.W. Ascaroside Signaling Is Widely Conserved among Nematodes. Curr. Biol. 2012, 22, 772-780.

40. Choe, A.; Chuman, T.; von Reuss, S.H.; Dossey, A.T.; Yim, J.J.; Ajredini, R.; Kolawa, A.A.; Kaplan, F.; Alborn, H.T.; Teal, P.E.A.; et al. Sex-specific mating pheromones in the nematode Panagrellus redivivus. Proc. Natl. Acad. Sci. USA 2012, 109, 20949-20954.

41. Dong, C.; Dolke, F.; Reuss, S.H. von Selective MS screening reveals a sex pheromone in Caenorhabditis briggsae and species-specificity in indole ascaroside signalling. Org. Biomol. Chem. 2016, 14, 7217-7225.

42. Dong, C.; Reilly, D.K.; Bergame, C.; Dolke, F.; Srinivasan, J.; von Reuss, S.H. Comparative Ascaroside Profiling of Caenorhabditis Exometabolomes Reveals Species-Specific (ω) and (ω-2)-Hydroxylation Downstream of Peroxisomal β-Oxidation. J. Org. Chem. 2018, 83, 7109-7120.

43. Izrayelit, Y.; Robinette, S.L.; Bose, N.; von Reuss, S.H.; Schroeder, F.C. 2D NMR-Based Metabolomics Uncovers Interactions between Conserved Biochemical Pathways in the Model Organism Caenorhabditis elegans. ACS Chem. Biol. 2013, 8, 314-319.

44. Zagoriy, V.; Matyash, V.; Kurzchalia, T. Long-Chain O-Ascarosyl-alkanediols Are Constitutive Components of Caenorhabditis elegans but Do Not Induce Dauer Larva Formation. Chem. Biodivers. 2010, 7, 2016-2022.

45. Griffiths, A.J.; Davies, D.B. Type-specific carbohydrate antigens of pathogenic bacteria. Part 1: Enterobacteriaceae. Carbohydr. Polym. 1991, 14, 241-279.

46. Thorson, J.S.; Lo, S.F.; Liu, H.W.; Hutchinson, C.R. Biosynthesis of 3, 6-dideoxyhexoses: New mechanistic reflections upon 2, 6-dideoxy, 4, 6-dideoxy, and amino sugar construction. J. Am. Chem. Soc. 1993, 115, 6993-6994.

47. Thorson, J.S.; Lo, S.F.; Ploux, O.; He, X.; Liu, H.W. Studies of the biosynthesis of 3,6-dideoxyhexoses: Molecular cloning and characterization of the asc (ascarylose) region from Yersinia pseudotuberculosis serogroup VA. J. Bacteriol. 1994, 176, 5483-5493.

48. Trefzer, A.; Bechthold, A.; Salas, J.A. Genes and enzymes involved in deoxysugar biosynthesis in bacteria. Nat. Prod. Rep. 1999, 16, 283-299.

49. Olson, S.K.; Greenan, G.; Desai, A.; Müller-Reichert, T.; Oegema, K. Hierarchical assembly of the eggshell and permeability barrier in C. elegans. J. Cell Biol 2012, 198, 731-748.

50. Campbell, J.A.; Davies, G.J.; Bulone, V.; Henrissat, B. A classification of nucleotide-diphospho-sugar glycosyltransferases based on amino acid sequence similarities. Biochem. J. 1997, 326, 929-939.

51. Koeller, K.M.; Wong, C.-H. Synthesis of complex carbohydrates and glycoconjugates: Enzyme-based and programmable one-pot strategies. Chem. Rev. 2000, 100, 4465-4494.

52. Gems, D.; McElwee, J.J. Broad spectrum detoxification: The major longevity assurance process regulated by insulin/IGF-1 signaling? Mech. Ageing Dev. 2005, 126, 381-387.

53. Lindblom, T.H.; Dodd, A.K. Xenobiotic detoxification in the nematode Caenorhabditis elegans. J. Exp. Zoolog. A Comp. Exp. Biol. 2006, 305A, 720-730.

54. Tukey, R.H.; Strassburg, C.P. Human UDP-Glucuronosyltransferases: Metabolism, Expression, and Disease. Annu. Rev. Pharmacol. Toxicol. 2000, 40, 581-616.

55. Artyukhin, A.B.; Yim, J.J.; Srinivasan, J.; Izrayelit, Y.; Bose, N.; von Reuss, S.H.; Jo, Y.; Jordan, J.M.; Baugh, L.R.; Cheong, M.; et al. Succinylated Octopamine Ascarosides and a New Pathway of Biogenic Amine Metabolism in Caenorhabditis elegans. J. Biol. Chem. 2013, 288, 18778-18783.

56. Motley, A.M.; Hettema, E.H.; Ketting, R.; Plasterk, R.; Tabak, H.F. Caenorhabditis elegans has a single pathway to target matrix proteins to peroxisomes. EMBO Rep. 2000, 1, 40-46.

57. Yokota, S.; Togo, S.H.; Maebuchi, M.; Bun-ya, M.; Haraguchi, C.M.; Kamiryo, T. Peroxisomes of the nematode Caenorhabditis elegans: Distribution and morphological characteristics. Histochem. Cell Biol. 2002, 118, 329-336.

58. Von Reuss, S.H. Exploring Modular Glycolipids Involved in Nematode Chemical Communication. CHIMIA Int. J. Chem. 2018, 72, 297-303.

59. Kim, K.-Y.; Joo, H.-J.; Kwon, H.-W.; Kim, H.; Hancock, W.S.; Paik, Y.-K. Development of a method to quantitate nematode pheromone for study of small-molecule metabolism in Caenorhabditis elegans. Anal. Chem. 2013, 85, 2681-2688.

60. Kaplan, F.; Srinivasan, J.; Mahanti, P.; Ajredini, R.; Durak, O.; Nimalendran, R.; Sternberg, P.W.; Teal, P.E.A.; Schroeder, F.C.; Edison, A.S.; et al. Ascaroside expression in Caenorhabditis elegans is strongly dependent on diet and developmental stage. PloS ONE 2011, 6, e17804.

61. Greene, J.S.; Brown, M.; Dobosiewicz, M.; Ishida, I.G.; Macosko, E.Z.; Zhang, X.; Butcher, R.A.; Cline, D.J.; McGrath, P.T.; Bargmann, C.I. Balancing selection shapes density-dependent foraging behaviour. Nature 2016, 539, 254-258.

62. Macosko, E.Z.; Pokala, N.; Feinberg, E.H.; Chalasani, S.H.; Butcher, R.A.; Clardy, J.; Bargmann, C.I. A hub-and-spoke circuit drives pheromone attraction and social behaviour in C. elegans. Nature 2009, 458, 1171-1175.

63. Jeong, P.-Y.; Kwon, M.-S.; Joo, H.-J.; Paik, Y.-K. Molecular Time-Course and the Metabolic Basis of Entry into Dauer in Caenorhabditis elegans. PLOS ONE 2009, 4, e4162.

64. Jones, S.J.M.; Riddle, D.L.; Pouzyrev, A.T.; Velculescu, V.E.; Hillier, L.; Eddy, S.R.; Stricklin, S.L.; Baillie, D.L.; Waterston, R.; Marra, M.A. Changes in Gene Expression Associated with Developmental Arrest and Longevity in Caenorhabditis elegans. Genome Res. 2001, 11, 1346-1352.

65. Wadsworth, W.G.; Riddle, D.L. Developmental regulation of energy metabolism in Caenorhabditis elegans. Dev. Biol. 1989, 132, 167-173.

66. Wang, J.; Kim, S.K. Global analysis of dauer gene expression in Caenorhabditis elegans. Development 2003, 130, 1621-1634.

67. Lee, H.; Choi, M.; Lee, D.; Kim, H.; Hwang, H.; Kim, H.; Park, S.; Paik, Y.; Lee, J. Nictation, a dispersal behavior of the nematode Caenorhabditis elegans, is regulated by IL2 neurons. Nat. Neurosci. 2012, 15, 107-112.

68. Lee, D.; Yang, H.; Kim, J.; Brady, S.; Zdraljevic, S.; Zamanian, M.; Kim, H.; Paik, Y.; Kruglyak, L.; Andersen, E.C.; et al. The genetic basis of natural variation in a phoretic behavior. Nat. Commun. 2017, 8, 273.

69. Kim, K.; Sato, K.; Shibuya, M.; Zeiger, D.M.; Butcher, R.A.; Ragains, J.R.; Clardy, J.; Touhara, K.; Sengupta, P. Two chemoreceptors mediate developmental effects of dauer pheromone in C. elegans. Science 2009, 326, 994-998.

70. Sommer, R.J.; Ogawa, A. Hormone Signaling and Phenotypic Plasticity in Nematode Development and Evolution. Curr. Biol. 2011, 21, R758-R766.

71. McGrath, P.T.; Xu, Y.; Ailion, M.; Garrison, J.L.; Butcher, R.A.; Bargmann, C.I. Parallel evolution of domesticated Caenorhabditis species targets pheromone receptor genes. Nature 2011, 477, 321-325.

72. Park, D.; O'Doherty, I.; Somvanshi, R.K.; Bethke, A.; Schroeder, F.C.; Kumar, U.; Riddle, D.L. Interaction of structure-specific and promiscuous G-protein-coupled receptors mediates small-molecule signaling in Caenorhabditis elegans. Proc. Natl. Acad. Sci. USA 2012, 109, 9917-9922.

73. Neal, S.J.; Park, J.; DiTirro, D.; Yoon, J.; Shibuya, M.; Choi, W.; Schroeder, F.C.; Butcher, R.A.; Kim, K.; Sengupta, P. A Forward Genetic Screen for Molecules Involved in Pheromone-Induced Dauer Formation in Caenorhabditis elegans. G3 Genes Genomes Genet. 2016, 6, 1475-1487.

74. Park, J.; Choi, W.; Dar, A.R.; Butcher, R.A.; Kim, K. Neuropeptide Signaling Regulates Pheromone-Mediated Gene Expression of a Chemoreceptor Gene in C. elegans. Mol. Cells 2018, 42, 28-35.

75. Ludewig, A.H.; Izrayelit, Y.; Park, D.; Malik, R.U.; Zimmermann, A.; Mahanti, P.; Fox, B.W.; Bethke, A.; Doering, F.; Riddle, D.L.; et al. Pheromone sensing regulates Caenorhabditis elegans lifespan and stress resistance via the deacetylase SIR-2.1. Proc. Natl. Acad. Sci. USA 2013, 110, 5522-5527.

76. Narayan, A.; Venkatachalam, V.; Durak, O.; Reilly, D.K.; Bose, N.; Schroeder, F.C.; Samuel, A.D.T.; Srinivasan, J.; Sternberg, P.W. Contrasting responses within a single neuron class enable sex-specific attraction in Caenorhabditis elegans. Proc. Natl. Acad. Sci. USA 2016, 113, E1392-E1401.

77. Fagan, K.A.; Luo, J.; Lagoy, R.C.; Schroeder, F.C.; Albrecht, D.R.; Portman, D.S. A Single-Neuron Chemosensory Switch Determines the Valence of a Sexually Dimorphic Sensory Behavior. Curr. Biol. 2018, 28, 902-914.

78. Park, D.; Hahm, J.-H.; Park, S.; Ha, G.; Chang, G.-E.; Jeong, H.; Kim, H.; Kim, S.; Cheong, E.; Paik, Y.-K. A conserved neuronal DAF-16/FoxO plays an important role in conveying pheromone signals to elicit repulsion behavior in Caenorhabditis elegans. Sci. Rep. 2017, 7, 7260.

79. Hong, M.; Ryu, L.; Ow, M.C.; Kim, J.; Je, A.R.; Chinta, S.; Huh, Y.H.; Lee, K.J.; Butcher, R.A.; Choi, H.; et al. Early Pheromone Experience Modifies a Synaptic Activity to Influence Adult Pheromone Responses of C. elegans. Curr. Biol. 2017, 27, 3168-3177.

80. Ryu, L.; Cheon, Y.; Huh, Y.H.; Pyo, S.; Chinta, S.; Choi, H.; Butcher, R.A.; Kim, K. Feeding state regulates pheromone-mediated avoidance behavior via the insulin signaling pathway in Caenorhabditis elegans. EMBO J. 2018, 37, e98402.

81. Zhang, Y.K.; Sanchez-Ayala, M.A.; Sternberg, P.W.; Srinivasan, J.; Schroeder, F.C. Improved Synthesis for Modular Ascarosides Uncovers Biological Activity. Org. Lett. 2017, 19, 2837-2840.

82. Fenk, L.A.; Bono, M. de Memory of recent oxygen experience switches pheromone valence in Caenorhabditis elegans. Proc. Natl. Acad. Sci. USA 2017, 114, 4195-4200.

83. Greene, J.S.; Dobosiewicz, M.; Butcher, R.A.; McGrath, P.T.; Bargmann, C.I. Regulatory changes in two chemoreceptor genes contribute to a Caenorhabditis elegans QTL for foraging behavior. eLife 2016, 5, e21454.

84. Bell, G. The Masterpiece of Nature: The Evolution and Genetics of Sexuality; CUP Archive: Cambridge, UK, 1982.

85. Dacks, J.; Roger, A.J. The First Sexual Lineage and the Relevance of Facultative Sex. J. Mol. Evol. 1999, 48, 779-783.

86. Dubnau, D. Genetic competence in Bacillus subtilis. Microbiol. Mol. Biol. Rev. 1991, 55, 395-424.

87. Gemmill, A.W.; Viney, M.E.; Read, A.F. Host Immune Status Determines Sexuality in a Parasitic Nematode. Evolution 1997, 51, 393-401.

88. Harris, E.H.; Stern, D.B.; Witman, G.B. The Chlamydomonas Sourcebook; Elsevier: San Diego, CA, USA, 2009.

89. Kleiven, O.T.; Larsson, P.; Hobæk, A. Sexual reproduction in Daphnia magna requires three stimuli. Oikos 1992, 197-206.

90. Lynch, M.; Bürger, R.; Butcher, D.; Gabriel, W. The Mutational Meltdown in Asexual Populations. J. Hered. 1993, 84, 339-344.

91. Mai, B.; Breeden, L. CLN1 and Its Repression by Xbp1 Are Important for Efficient Sporulation in Budding Yeast. Mol. Cell. Biol. 2000, 20, 478-487.

92. Muller, H.J. The relation of recombination to mutational advance. Mutat. Res. Mol. Mech. Mutagen. 1964, 1, 2-9.

93. Morran, L.T.; Cappy, B.J.; Anderson, J.L.; Phillips, P.C. Sexual Partners for the Stressed: Facultative Outcrossing in the Self-Fertilizing Nematode Caenorhabditis Elegans. Evolution 2009, 63, 1473-1482.

94. Wharam, B.; Weldon, L.; Viney, M. Pheromone modulates two phenotypically plastic traits-adult reproduction and larval diapause-In the nematode Caenorhabditis elegans. BMC Evol. Biol. 2017, 17, 197.

95. Izrayelit, Y.; Srinivasan, J.; Campbell, S.L.; Jo, Y.; von Reuss, S.H.; Genoff, M.C.; Sternberg, P.W.; Schroeder, F.C. Targeted Metabolomics Reveals a Male Pheromone and Sex-Specific Ascaroside Biosynthesis in Caenorhabditis elegans. ACS Chem. Biol. 2012, 7, 1321-1325.

96. Aprison, E.Z.; Ruvinsky, I. Sex Pheromones of C. elegans Males Prime the Female Reproductive System and Ameliorate the Effects of Heat Stress. PLOS Genet. 2015, 11, e1005729.

97. Shi, C.; Runnels, A.M.; Murphy, C.T. Mating and male pheromone kill Caenorhabditis males through distinct mechanisms. eLife. 2017, 6, e23493.

98. Riddle, D.L.; Blumenthal, T.; Meyer, B.J.; Priess, J.R. C. elegans II, 2nd ed.; Cold Spring Harbor Laboratory Press: Cold Spring Harbor, NY, USA, 1997.

99. Berger, J.; Dorninger, F.; Forss-Petter, S.; Kunze, M. Peroxisomes in brain development and function. Biochim. Biophys. Acta BBA-Mol. Cell Res. 2016, 1863, 934-955.

100. Clayton, P.T. Clinical consequences of defects in peroxisomal β-oxidation. Biochem. Soc. Trans. 2001, 29, 298-305.

101. Crane, D.I. Revisiting the neuropathogenesis of Zellweger syndrome. Neurochem. Int. 2014, 69, 1-8.

102. De Munter, S.; Verheijden, S.; Régal, L.; Baes, M. Peroxisomal Disorders: A Review on Cerebellar Pathologies. Brain Pathol. 2015, 25, 663-678.

103. Wanders, R.J.A. Peroxisomes, lipid metabolism, and peroxisomal disorders. Mol. Genet. Metab. 2004, 83, 16-27.

104. Wanders, R.J.A.; Waterham, H.R. Peroxisomal disorders: The single peroxisomal enzyme deficiencies. Biochim. Biophys. Acta BBA-Mol. Cell Res. 2006, 1763, 1707-1720.

105. Brites, P.; Mooyer, P.A.W.; el Mrabet, L.; Waterham, H.R.; Wanders, R.J.A. Plasmalogens participate in very-long-chain fatty acid-induced pathology. Brain 2009, 132, 482-492.

106. Trompier, D.; Vejux, A.; Zarrouk, A.; Gondcaille, C.; Geillon, F.; Nury, T.; Savary, S.; Lizard, G. Brain peroxisomes. Biochimie 2014, 98, 102-110.

107. Park, S.; Paik, Y.-K. Genetic deficiency in neuronal peroxisomal fatty acid β-oxidation causes the interruption of dauer development in Caenorhabditis elegans. Sci. Rep. 2017, 7, 9358.

108. Kulalert, W.; Kim, D.H. The Unfolded Protein Response in a Pair of Sensory Neurons Promotes Entry of C. elegans into Dauer Diapause. Curr. Biol. 2013, 23, 2540-2545.

109. Malone, E.A.; Thomas, J.H. A screen for nonconditional dauer-constitutive mutations in Caenorhabditis elegans. Genetics 1994, 136, 879-886.

110. Li, W.; Kennedy, S.G.; Ruvkun, G. daf-28 encodes a C. elegans insulin superfamily member that is regulated by environmental cues and acts in the DAF-2 signaling pathway. Genes Dev. 2003, 17, 844-858.

111. Kulalert, W.; Sadeeshkumar, H.; Zhang, Y.K.; Schroeder, F.C.; Kim, D.H. Molecular Determinants of the Regulation of Development and Metabolism by Neuronal eIF2α Phosphorylation in Caenorhabditis elegans. Genetics 2017, 206, 251-263.

112. Ludewig, A. Ascaroside signaling in C. elegans. WormBook 2013, 1-22.

113. Neal, S.J.; Takeishi, A.; O'Donnell, M.P.; Park, J.; Hong, M.; Butcher, R.A.; Kim, K.; Sengupta, P. Feeding state-dependent regulation of developmental plasticity via CaMKI and neuroendocrine signaling. eLife 2015, 4, e10110.

114. O'Donnell, M.P.; Chao, P.-H.; Kammenga, J.E.; Sengupta, P. Rictor/TORC2 mediates gut-to-brain signaling in the regulation of phenotypic plasticity in C. elegans. PLOS Genet. 2018, 14, e1007213.

115. Ilbay, O.; Ambros, V. Pheromones and Nutritional Signals Regulate the Developmental Reliance on let-7 Family MicroRNAs in C. elegans. Curr. Biol. 2019, 29, 1735-1745.

116. Yamada, K.; Hirotsu, T.; Matsuki, M.; Butcher, R.A.; Tomioka, M.; Ishihara, T.; Clardy, J.; Kunitomo, H.; Iino, Y. Olfactory Plasticity Is Regulated by Pheromonal Signaling in Caenorhabditis elegans. Science 2010, 329, 1647-1650.

117. Fielenbach, N.; Antebi, A.C. elegans dauer formation and the molecular basis of plasticity. Genes Dev. 2008, 22, 2149-2165.

118. Hahm, J.-H.; Kim, S.; Paik, Y.-K. Endogenous cGMP regulates adult longevity via the insulin signaling pathway in Caenorhabditis elegans. Aging Cell 2009, 8, 473-483.

119. Artan, M.; Jeong, D.-E.; Lee, D.; Kim, Y.-I.; Son, H.G.; Husain, Z.; Kim, J.; Altintas, O.; Kim, K.; Alcedo, J.; et al. Food-derived sensory cues modulate longevity via distinct neuroendocrine insulin-like peptides. Genes Dev. 2016, 30, 1047-1057.

120. Fletcher, M.; Kim, D.H. Age-Dependent Neuroendocrine Signaling from Sensory Neurons Modulates the Effect of Dietary Restriction on Longevity of Caenorhabditis elegans. PLOS Genet. 2017, 13, e1006544.

121. Ludewig, A.H.; Gimond, C.; Judkins, J.C.; Thornton, S.; Pulido, D.C.; Micikas, R.J.; Döring, F.; Antebi, A.; Braendle, C.; Schroeder, F.C. Larval crowding accelerates C. elegans development and reduces lifespan. PLOS Genet. 2017, 13, e1006717.

122. Schulenburg, H.; Ewbank, J.J. The genetics of pathogen avoidance in Caenorhabditis elegans. Mol. Microbiol. 2007, 66, 563-570.

123. Meisel, J.D.; Kim, D.H. Behavioral avoidance of pathogenic bacteria by Caenorhabditis elegans. Trends Immunol. 2014, 35, 465-470.

124. Kim, D.H. Bacteria and the Aging and Longevity of Caenorhabditis elegans. Annu. Rev. Genet. 2013, 47, 233-246.

125. Reddy, K.C.; Andersen, E.C.; Kruglyak, L.; Kim, D.H. A Polymorphism in npr-1 Is a Behavioral Determinant of Pathogen Susceptibility in C. elegans. Science 2009, 323, 382-384.

126. Reddy, K.C.; Hunter, R.C.; Bhatla, N.; Newman, D.K.; Kim, D.H. Caenorhabditis elegans NPR-1-mediated behaviors are suppressed in the presence of mucoid bacteria. Proc. Natl. Acad. Sci. USA 2011, 108, 12887-12892.

127. Styer, K.L.; Singh, V.; Macosko, E.; Steele, S.E.; Bargmann, C.I.; Aballay, A. Innate Immunity in Caenorhabditis elegans Is Regulated by Neurons Expressing NPR-1/GPCR. Science 2008, 322, 460-464.

128. Chang, H.C.; Paek, J.; Kim, D.H. Natural polymorphisms in C. elegans HECW-1 E3 ligase affect pathogen avoidance behaviour. Nature 2011, 480, 525-529.

129. Cao, X.; Kajino-Sakamoto, R.; Doss, A.; Aballay, A. Distinct Roles of Sensory Neurons in Mediating Pathogen Avoidance and Neuropeptide-Dependent Immune Regulation. Cell Rep. 2017, 21, 1442-1451.

130. Meisel, J.D.; Panda, O.; Mahanti, P.; Schroeder, F.C.; Kim, D.H. Chemosensation of Bacterial Secondary Metabolites Modulates Neuroendocrine Signaling and Behavior of C. elegans. Cell 2014, 159, 267-280.

131. Moore, R.S.; Kaletsky, R.; Murphy, C.T. Piwi/PRG-1 Argonaute and TGF-β Mediate Transgenerational Learned Pathogenic Avoidance. Cell 2019, 177, 1827-1841.

132. Lee, K.; Mylonakis, E. An Intestine-Derived Neuropeptide Controls Avoidance Behavior in Caenorhabditis elegans. Cell Rep. 2017, 20, 2501-2512.

133. Richardson, C.E.; Kooistra, T.; Kim, D.H. An essential role for XBP-1 in host protection against immune activation in C. elegans. Nature 2010, 463, 1092-1095.

134. Richardson, C.E.; Kinkel, S.; Kim, D.H. Physiological IRE-1-XBP-1 and PEK-1 Signaling in Caenorhabditis elegans Larval Development and Immunity. PLOS Genet. 2011, 7, e1002391.

135. Sun, J.; Liu, Y.; Aballay, A. Organismal regulation of XBP-1-mediated unfolded protein response during development and immune activation. EMBO Rep. 2012, 13, 855-860.

136. Sun, J.; Singh, V.; Kajino-Sakamoto, R.; Aballay, A. Neuronal GPCR Controls Innate Immunity by Regulating Noncanonical Unfolded Protein Response Genes. Science 2011, 332, 729-732.

137. Park, J.H.; Chung, H.Y.; Kim, M.; Lee, J.H.; Jung, M.; Ha, H. Daumone fed late in life improves survival and reduces hepatic inflammation and fibrosis in mice. Aging Cell 2014, 13, 709-718.

138. Park, J.H.; Ha, H. Short-term Treatment of Daumone Improves Hepatic Inflammation in Aged Mice. Korean J. Physiol. Pharmacol. 2015, 19, 269.

139. Ma, G.T.; Lee, S.K.; Park, K.-K.; Park, J.; Son, S.H.; Jung, M.; Chung, W.-Y. Artemisinin-Daumone Hybrid Inhibits Cancer Cell-Mediated Osteolysis by Targeting Cancer Cells and Osteoclasts. Cell. Physiol. Biochem. 2018, 49, 1460-1475.

140. Consortium, T.C. elegans S. Genome Sequence of the Nematode C. elegans: A Platform for Investigating Biology. Science 1998, 282, 2012-2018.

141. Nagarathnam, B.; Kalaimathy, S.; Balakrishnan, V.; Sowdhamini, R. Cross-Genome Clustering of Human and C. elegans G-Protein Coupled Receptors. Evol. Bioinforma. 2012, 8, EBO-S9405.