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Brief Funct Genomics. 2011 July; 10(4): 175–180.
Published online 2011 May 29. doi:  10.1093/bfgp/elr012
PMCID: PMC3144738

A growing molecular toolbox for the functional analysis of microRNAs in Caenorhabditis elegans


With the growing number of microRNAs (miRNAs) being identified each year, more innovative molecular tools are required to efficiently characterize these small RNAs in living animal systems. Caenorhabditis elegans is a powerful model to study how miRNAs regulate gene expression and control diverse biological processes during development and in the adult. Genetic strategies such as large-scale miRNA deletion studies in nematodes have been used with limited success since the majority of miRNA genes do not exhibit phenotypes when individually mutated. Recent work has indicated that miRNAs function in complex regulatory networks with other small RNAs and protein-coding genes, and therefore the challenge will be to uncover these functional redundancies. The use of miRNA inhibitors such as synthetic antisense 2′-O-methyl oligoribonucleotides is emerging as a promising in vivo approach to dissect out the intricacies of miRNA regulation.

Keywords: microRNA, Caenorhabditis elegans, miRNA inhibitors, antisense 2′-O-methyl oligoribonucleotides

MicroRNAs (miRNAs) belong to a large class of small non-coding RNAs that have captured the attention of scientists and clinicians alike due to their importance during animal development and their close correlation to human disorders such as cancer [1, 2]. MiRNAs are extensively processed in the nucleus and the cytoplasm by the RNase III enzymes Drosha and Dicer, respectively, before generating the mature single-stranded ~22-nt RNA species [3]. MiRNAs are subsequently loaded into a large multi-protein miRNA ribonucleoprotein complex (miRNP) and function to negatively regulate gene expression by associating in a sequence-specific manner typically within the 3′-untranslated region (3′-UTR) of their target messenger RNA (mRNA) transcripts resulting in translational inhibition and/or mRNA degradation [4]. Animal miRNAs bind to their targets with incomplete complementarity and this interaction allows for bulges, loops and G-U base pairing to occur outside of the miRNA ‘seed’ region (nt 2–8 of the miRNA that generally bind perfectly with its target). The founding members of the miRNA family, lin-4 and let-7, were first identified in Caenorhabditis elegans via forward genetic screens and found to act as ‘developmental switches’ that control the timing of the larval and adult transitions [5–7]. Since this discovery, thousands of miRNA genes have been identified in various organisms ranging from insects, fish, birds, mammals, plants and viruses by primarily using small RNA cloning, deep sequencing and bioinformatic approaches [8]. While the number of miRNAs identified continues to climb (approximately 1424 miRNA genes have been validated in the human genome thus far), our ability to tease out their biological roles in the intact organism has lagged behind. Indeed, only a fraction of animal miRNAs have been well-characterized and are found to direct essential events related to cellular differentiation, proliferation, immune surveillance, metabolism and lifespan [1].

A major challenge in the field is to devise high-throughput methods to determine the functional significance of miRNA genes as well as identify the targets that these small RNAs control. Target identification is difficult due to the imperfect association of the miRNA to the mRNA target and current tools such as computational prediction algorithms and microarray analysis result in high false positive and false negative rates. This issue is compounded by the fact that a single miRNA can regulate the expression of multiple mRNA targets and therefore can modulate distinct genetic pathways simultaneously. Innovative experimental tools are required to understand the biological roles of miRNAs within and across closely related RNA families in the intact animal and to probe how certain miRNAs function in complex biological networks with other non-coding RNAs and protein coding genes during development and in the adult.

Use of the simple and genetically amenable C. elegans animal model has been extremely successful in studying miRNA regulation and function (Table 1). Genome-wide RNAi suppressor screens performed in miRNA loss-of-function mutant backgrounds [9] and pull-down assays to identify mRNA targets loaded into miRNP complexes [Argonaut (ALG-1) HITS-CLIP screens] [10, 11] have provided insight into the multitude of mRNA targets controlled by small RNAs. The generation of animals carrying transgenic arrays consisting of miRNA promoter elements driving green fluorescent protein (GFP) expression has been a valuable method to determine the in vivo spatial and temporal expression patterns of miRNAs throughout development and discern biological activity [12–16]. C. elegans overexpression studies that employ extrachromosomal arrays expressing transgenes for individual miRNAs such as lin-4, let-7, mir-48, mir-61 and mir-84 result in obvious phenotypes that have aided in the characterization of their functional roles [7, 17–21]. However, ectopic expression of miRNAs in general can result in a bias to downregulate artificial targets or drive miRNA expression at the wrong time or place compared to wild-type expression patterns making the phenotypes observed difficult to interpret. These studies (as well as miRNA promoter::GFP expression studies described above) are also hindered by the fact that high-copy transgenic arrays are not expressed in the germ line. Therefore, the use of specialized techniques to achieve single/low copy expression such as microparticle bombardment or Mos1 mediated Single Copy transgene Insertion (MosSCI) would be required for the analysis of miRNAs in this tissue [22, 23].

Table 1:
Current in vivo methods to investigate miRNA function in C. elegans

Large scale deletion studies in C. elegans have revealed that with the exception of lin-4 [6], let-7 [7], lsy-6 [12] and mir-1 [24], individual elimination of 91 additional miRNAs fail to produce overt phenotypes [25]. These results indicate that the majority of miRNA genes are individually not crucial for viability or developmental processes and that many miRNAs likely possess redundant functions. In support of this notion, recent work has shown that in the case of the mir-35, mir-51, mir-58 and let-7 families in C. elegans, multiple closely related miRNA members sharing identical ‘seed’ sequences must be deleted in combination in order to uncover gross morphological abnormalities and embryonic lethal phenotypes [26–28]. Interestingly, Alarez-Saavedra and Horvitz [26] found that for 12 additional miRNA families tested in the worm, the deletion of multiple miRNA members within these individual families failed to produce any measurable defects and therefore the authors concluded that most miRNAs are not essential and do not regulate important developmental functions. In contrast, Brenner and colleagues showed that loss of 25 out of 31 individual miRNAs assayed in sensitized genetic backgrounds, such as alg-1 loss-of-function mutants, resulted in obvious mutant phenotypes and implies that functional redundancies must exist between certain miRNAs, across individual miRNA families or with other non-miRNA genes [29]. Taken together, these miRNA deletion studies have been hampered by a lack of phenotypes observed when miRNAs are individually eliminated due in part to functional redundancies as well as the difficulties in interpreting embryonic lethal and sterile phenotypes. This approach also has limitations when attempting to study miRNA genes that exist in clusters, which often share common promoter elements, or miRNAs located within introns of protein-coding genes, since deletion mutations in these sites could alter the function of multiple genes.

Given the shortcomings of currently available technologies, additional methods are needed to interrogate miRNA activity in vivo within biological networks, at specific stages of development, under certain environmental conditions as well as in specific cell populations of the worm in order to determine their biological roles. Fortunately, Zheng and colleagues have recently added another reagent to the C. elegans toolbox that can potentially address many of these issues—the development of dextran-conjugated antisense 2′-O-methyl oligoribonucleotides that block miRNA activity within the living animal by competitively binding to endogenous miRNAs and preventing association with their mRNA targets [30].

Zheng’s group recognized that C. elegans researchers lacked an effective method to experimentally inactivate miRNAs in nematodes throughout various stages of development. The ideal reagent would need to be resistant to degradation, potent at low concentrations, nontoxic to the developing animal and possess high specificity to block the activity of individual miRNAs without cross-reacting with closely related miRNA family members. Furthermore, the miRNA inhibitors would be most useful in functional assays if they could be mixed into ‘cocktails’ in which select miRNAs could be inactivated in groups to uncover functional redundancies. Hutvagner and colleagues [31] first described the use of antisense oligoribonucleotides to inactivate miRNAs in C. elegans 6 years ago. In this early study, oligonucleotides carrying 2′-O-methyl modifications (to prevent degradation by nucleases) and antisense to let-7 were injected directly into the body cavity of early larval stage (L2/L3) animals resulting in hypodermal defects and bursting vulval phenotypes that resembled abnormalities observed in let-7 deletion mutants [7] (Figure 1, left panel). Although promising, these first-generation C. elegans miRNA inhibitors could not produce phenotypes in the progeny of adult animals injected within the germ line. This approach requires the injection of antisense oligonucleotides into individual larval stage nematodes, which is extremely laborious, technologically challenging and impossible to use to study miRNA function in the embryo and at early larval stages of development. Zheng and colleagues [30] theorized that the miRNA inhibitors used by Hutvagner’s group were not transmitted to the progeny of the injected animals due to poor uptake and cellular retention. To circumvent these problems, the authors conjugated one, four or eight copies of 2′-O-methyl oligoribonucleotides antisense to specific miRNAs with dextran, a nontoxic polysaccharide that is highly soluble and well retained in cells (Figure 1, right panel). These dextran-conjugated miRNA inhibitors were also labeled with a fluorescent rhodamine marker to allow the researchers to track phenotypes only in animals successfully delivered the reagent.

Figure 1:
Antisense 2′-O-methyl oligonucleotides are effective agents to block miRNA activity in C. elegans. (A) Hutvanger and colleagues [31] devised first generation antisense 2′-O-methyl (Me) oligonucleotides (oligos) against let-7 that can be ...

As a proof-of-principle experiment, Zheng and his group injected the syncytial germ line of adult hermaphrodites with dextran-conjugated oligoribonucleotides antisense to lin-4 [30]. Loss-of-function phenotypes for lin-4 have been well characterized and include complete absence of egg-laying structures (the vulvaless phenotype), reiteration of early larval division patterns in the hypodermal seam cells and absence of adult alae formation in the nematode [5, 6]. The authors found that progeny carrying dextran reagents conjugated with one or four copies of the antisense lin-4 2′-O-methyl oligoribonucleotide exhibited potent inhibition of lin-4 activity (100% showed egg-laying defects at 20 µM). Importantly, injection of C. elegans with dextran-conjugated oligoribonucleotides antisense to the highly homologous lin-4 family member mir-237 did not result in egg-laying defects or any other obvious abnormalities, mirroring the lack of phenotypes reported in animals genetically deleted for miR-237 [25] and demonstrating the high specificity of the antisense reagent.

This technique holds great promise as a powerful in vivo experimental tool that can be applied to a large range of miRNA genes. Indeed, Zheng et al. [30] found that the use of dextran-conjugated antisense oligoribonucleotides blocked the activity of three additional well-characterized miRNAs, let-7, required for the L4-to-adult transition in hypodermal cells, lsy-6, essential for left–right patterning of chemosensory ASE neurons, and mir-42, a member of the mir-35 family that is expressed only during embryogenesis. Moreover, the dextran-conjugated antisense oligoribonucleotides could be used in combination to inhibit the activity of multiple miRNAs in a single experiment, as demonstrated when the authors co-injected reagents against lin-4 and lys-6 and observed both egg-laying abnormalities and ASE neuron patterning defects in all of the treated progeny.

These encouraging results indicate that the dextran moiety enables the miRNA inhibitors to be retained in the injected adult germ line as well as in the developing progeny. Furthermore, these antisense reagents are very specific for the miRNA being targeted since off-targeting effects were not observed. An important question, however, is how long does this miRNA inhibition last? Following injection of dextran-conjugated miRNA inhibitors to the worm, the reagent becomes diluted out with each cellular division and potentially is destabilized/degraded over time. Zheng and colleagues [30] addressed this question when they assayed lin-4 inhibition in treated progeny for suppressed expression of an adult hypodermal cell marker, col-19. The authors found that dextran-conjugated lin-4 inhibitors could only suppress miRNA activity (and thus col-19 expression) in the developing progeny ~10–15 h following the L4 larval molt and after this time lin-4 activity was present in the adult animals. This finding shows that miRNA inhibition with this reagent is temporally limited and unsuitable for studying miRNA function in treated adult progeny for processes such as fertility and aging. Furthermore, these dextran-conjugated antisense oligoribonucleotides do not appear to completely eliminate miRNA function in the hypodermis of treated progeny, even at the earliest larval stages. When characterizing another classic lin-4 loss-of-function phenotype, the reiteration of L1 larval fates in hypodermal seam cells, Zheng and colleagues noted that progeny treated with antisense lin-4 oligoribonucleotides exhibited a repeat of L2 larval division patterns (rather than L1 fates) in seam cells, suggesting that this miRNA was reduced but not absent in this tissue during early larval development. In terms of overall toxicity, high doses (>50 µM) of dextran-conjugated miRNA inhibitors injected into nematodes showed detrimental effects in the treated progeny, specifically increased embryonic lethality and egg-hatching defects.

Although dextran-conjugated antisense 2′-O-methyl oligoribonucleotides should be effective in characterizing the role of the 207 miRNA genes currently identified in the C. elegans genome, more work needs to be done to optimize these miRNA inhibitory-based tools. Synthetic antisense oligoribonucleotides that carry alternative RNA modifications to improve their stability such as phosphorothiaote linkages or locked nucleic acids (LNAs, 2′-O, 4′-C-methylene bridge), which are proven to be less toxic and more potent in mammalian systems, may be good alternatives for in vivo studies in C. elegans. Unfortunately, a significant disadvantage of using antisense technologies devised by the Hutvagner and Zheng groups for large-scale functional screens is the reliance of single worm microinjection to deliver these reagents to the animals in contrast to other methods, i.e. delivery by soaking. Existing miRNA inhibitor strategies in C. elegans are also not amenable to block miRNA activity in a cell type-specific manner, at certain times during the worm lifecycle or to assay effects in multiple generations.

Looking forward, this technology will likely move toward the generation of C. elegans carrying transgenes expressing miRNA sponges—a method devised by Ebert and colleagues for use in mammalian cells [32]. MiRNA sponges function as decoy targets to inhibit miRNA activity and consist of a tandem array of miRNA-binding sites engineered within the 3′-UTR of a reporter gene driven by a strong promoter. The miRNA complementary sites in the sponge constructs are mismatched for nt 8–11 of the mature miRNA sequence and allow stable binding and sequestering of the miRNA away from its endogenous targets. These miRNA sponges could be engineered to interrogate specific biological processes within the worm in both a temporal and spatial manner by regulating transgenic expression of the miRNA inhibitors using tissue specific or heat shock promoters or via conditional elements based on Cre, FLP or MEC-8-dependent splicing technologies [33–36]. Potentially, these inhibitors could even be designed to inhibit the activity of multiple miRNA genes. The future is bright for miRNA research and with a growing molecular toolbox available in C elegans, this model organism will undoubtedly remain at the forefront to interrogate miRNA networks in living systems.

Key Points

  • MicroRNAs (miRNAs) are ~22 nt non-coding RNAs that negatively regulate gene expression post-transcriptionally by binding to the 3′-UTRs of messenger RNA (mRNA) targets. Thousands of miRNAs have been identified in plant, animal and viral systems but only a small portion have been biologically characterized.
  • The C. elegans animal model has successfully been used for studying miRNA function and regulation. Molecular tools such as RNAi suppressor screens, miRNA promoter::GFP fusion constructs as well as overexpression and deletion analysis have been employed in vivo to determine the role of miRNAs during development in the nematode. These approaches possess technical limitations that make it difficult to elucidate the physiological significance of miRNAs or how they interact within intricate networks with other small RNAs and protein-coding genes.
  • Antisense 2′-O-methyl oligonucleotides are promising reagents that inhibit small RNA activity in the living nematode by physically binding to endogenous miRNAs and blocking their interaction with mRNA targets. Dextran-conjugated 2′-O-methyl oligoribonucleotides can inactivate multiple miRNAs in a single experiment and therefore could potentially be used to study functional redundancies. However, these miRNA inhibitors are laborious to deliver via single animal microinjection and have limited potency in treated progeny during the C. elegans lifecycle.
  • More innovative and high-throughput approaches are required to aid in the characterization of the >200 miRNAs that exist within the C. elegans genome. In the future, miRNA sponges could be adapted to inhibit C. elegans miRNA activity in a temporal and spatial manner.


The National Institutes of Health and the National Cancer Institute (RO3 CA139547 & R21 CA137704); the Thomas F. and Kate Miller Jeffress Memorial Trust and Eastern Virginia Medical School laboratory start-up funds to A. E. K.


The authors thank Helge Grosshans for critical reading of the manuscript.



Jeanyoung Jo received her BA in Biology from Wellesley College in Wellesley, Massachusetts and is a member of Dr Esquela-Kerscher’s laboratory in which she studies the role of miRNAs during development using the C. elegans animal model.


Aurora Esquela-Kerscher received her BA from Washington University in St Louis, Missouri and completed her MS in biotechnology and PhD in biochemistry, cellular and molecular biology at the Johns Hopkins University School of Medicine. She conducted her postdoctoral fellowship in Frank Slack’s laboratory at Yale University where she began her studies to determine how miRNAs control developmental events. She is currently an assistant professor in the Department of Microbiology and Molecular Cell Biology at Eastern Virginia Medical School and an adjunct assistant professor in the Department of Applied Science at the College of William and Mary.


1. Stefani G, Slack FJ. Small non-coding RNAs in animal development. Nat Rev Mol Cell Biol. 2008;9:219–30. [PubMed]
2. Esquela-Kerscher A, Slack FJ. Oncomirs - microRNAs with a role in cancer. Nat Rev Cancer. 2006;6:259–69. [PubMed]
3. Kim VN, Han J, Siomi MC. Biogenesis of small RNAs in animals. Nat Rev Mol Cell Biol. 2009;10:126–39. [PubMed]
4. Filipowicz W, Bhattacharyya SN, Sonenberg N. Mechanisms of post-transcriptional regulation by microRNAs: are the answers in sight? Nat Rev Genet. 2008;9:102–14. [PubMed]
5. Ambros V, Horvitz HR. Heterochronic mutants of the nematode. Caenorhabditis elegans. Science. 1984;226:409–16. [PubMed]
6. Lee RC, Feinbaum RL, Ambros V. The C. elegans heterochronic gene lin-4 encodes small RNAs with antisense complementarity to lin-14. Cell. 1993;75:843–54. [PubMed]
7. Reinhart B, Slack F, Basson M, et al. The 21 nucleotide let-7 RNA regulates C. elegans developmental timing. Nature. 2000;403:901–6. [PubMed]
8. Griffiths-Jones S, Saini HK, van Dongen S, et al. miRBase: tools for microRNA genomics. Nucleic Acids Res. 2008;36:D154–8. [PMC free article] [PubMed]
9. Grosshans H, Johnson T, Reinert KL, et al. The temporal patterning microRNA let-7 regulates several transcription factors at the larval to adult transition in C. elegans. Dev Cell. 2005;8:321–30. [PubMed]
10. Chi SW, Zang JB, Mele A, et al. Argonaute HITS-CLIP decodes microRNA-mRNA interaction maps. Nature. 2009;460:479–86. [PMC free article] [PubMed]
11. Zisoulis DG, Lovci MT, Wilbert ML, et al. Comprehensive discovery of endogenous Argonaute binding sites in Caenorhabditis elegans. Nat Struct Mol Biol. 2010;17:173–9. [PMC free article] [PubMed]
12. Johnston RJ, Hobert O. A microRNA controlling left/right neuronal asymmetry in Caenorhabditis elegans. Nature. 2003;426:845–9. [PubMed]
13. Isik M, Korswagen HC, Berezikov E. Expression patterns of intronic microRNAs in Caenorhabditis elegans. Silence. 2010;1:5. [PMC free article] [PubMed]
14. Martinez NJ, Ow MC, Reece-Hoyes JS, et al. Genome-scale spatiotemporal analysis of Caenorhabditis elegans microRNA promoter activity. Genome Res. 2008;18:2005–15. [PubMed]
15. Johnson SM, Lin SY, Slack FJ. The time of appearance of the C. elegans let-7 microRNA is transcriptionally controlled utilizing a temporal regulatory element in its promoter. Dev Biol. 2003;259:364–79. [PubMed]
16. Esquela-Kerscher A, Johnson SM, Bai L, et al. Post-embryonic expression of C. elegans microRNAs belonging to the lin-4 and let-7 families in the hypodermis and the reproductive system. Dev Dyn. 2005;234:868–77. [PMC free article] [PubMed]
17. Boehm M, Slack F. A developmental timing microRNA and its target regulate life span in C. elegans. Science. 2005;310:1954–7. [PubMed]
18. Feinbaum R, Ambros V. The timing of lin-4 RNA accumulation controls the timing of postembryonic developmental events in Caenorhabditis elegans. Dev Biol. 1999;210:87–95. [PubMed]
19. Johnson SM, Grosshans H, Shingara J, et al. RAS is regulated by the let-7 microRNA family. Cell. 2005;120:635–47. [PubMed]
20. Li M, Jones-Rhoades MW, Lau NC, et al. Regulatory mutations of mir-48, a C. elegans let-7 family MicroRNA, cause developmental timing defects. Dev Cell. 2005;9:415–22. [PubMed]
21. Yoo AS, Bais C, Greenwald I. Crosstalk between the EGFR and LIN-12/Notch pathways in C. elegans vulval development. Science. 2004;303:663–6. [PubMed]
22. Merritt C, et al. Transgenic solutions for the germline (February 8, 2010). In Wormbook (ed). The C. elegans Research Community, WormBook, doi:10.1895/wormbook.1.148.1,
23. Frokjaer-Jensen C, Davis MW, Hopkins CE, et al. Single-copy insertion of transgenes in Caenorhabditis elegans. Nat Genet. 2008;40:1375–83. [PMC free article] [PubMed]
24. Simon DJ, Madison JM, Conery AL, et al. The microRNA miR-1 regulates a MEF-2-dependent retrograde signal at neuromuscular junctions. Cell. 2008;133:903–15. [PMC free article] [PubMed]
25. Miska EA, Alvarez-Saavedra E, Abbott AL, et al. Most Caenorhabditis elegans microRNAs are individually not essential for development or viability. PLoS Genet. 2007;3:e215. [PubMed]
26. Alvarez-Saavedra E, Horvitz HR. Many families of C. elegans microRNAs are not essential for development or viability. Curr Biol. 2010;20:367–73. [PMC free article] [PubMed]
27. Abbott AL, Alvarez-Saavedra E, Miska EA, et al. The let-7 MicroRNA family members mir-48, mir-84, and mir-241 function together to regulate developmental timing in Caenorhabditis elegans. Dev Cell. 2005;9:403–14. [PubMed]
28. Shaw WR, Armisen J, Lehrbach NJ, et al. The Conserved miR-51 microRNA family is redundantly required for embryonic development and pharynx attachment in Caenorhabditis elegans. Genetics. 2010;185:897–905. [PubMed]
29. Brenner JL, Jasiewicz KL, Fahley AF, et al. Loss of individual microRNAs causes mutant phenotypes in sensitized genetic backgrounds in C. elegans. Curr Biol. 2010;20:1321–5. [PMC free article] [PubMed]
30. Zheng G, Ambros V, Li WH. Inhibiting miRNA in Caenorhabditis elegans using a potent and selective antisense reagent. Silence. 2010;1:9. [PMC free article] [PubMed]
31. Hutvagner G, Simard MJ, Mello CC, et al. Sequence-specific inhibition of small RNA function. PLoS Biol. 2004;2:E98. [PMC free article] [PubMed]
32. Ebert MS, Neilson JR, Sharp PA. MicroRNA sponges: competitive inhibitors of small RNAs in mammalian cells. Nat Methods. 2007;4:721–6. [PubMed]
33. Calixto A, Ma C, Chalfie M. Conditional gene expression and RNAi using MEC-8-dependent splicing in C. elegans. Nat Methods. 2010;7:407–11. [PMC free article] [PubMed]
34. Macosko EZ, Pokala N, Feinberg EH, et al. A hub-and-spoke circuit drives pheromone attraction and social behaviour in C. elegans. Nature. 2009;458:1171–5. [PMC free article] [PubMed]
35. Voutev R, Hubbard EJ. A "FLP-Out" system for controlled gene expression in Caenorhabditis elegans. Genetics. 2008;180:103–19. [PubMed]
36. Davis MW, Morton JJ, Carroll D, et al. Gene activation using FLP recombinase in C. elegans. PLoS Genet. 2008;4:e1000028. [PMC free article] [PubMed]

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