# Patent

## Title
Cloning sequencing and characterization of two cell death genes and uses therefor

## Abstract

Described herein are genes shown to be essential for programmed cell death in C. elegans, their encoded products (RNA and polypeptides), antibodies directed against the encoded polypeptides; probes for identifying structurally related genes and bioassays for identifying functionally related cell death genes from various organisms; methods and agents for altering (increasing or decreasing) the activity of the cell death-genes and, thus, of altering cell death; and uses therefor. Specifically, two genes shown to be essential for almost all of the cell deaths which occur in the development of C. elegans, referred to as ced-3 and ced-4, have been cloned, sequenced and characterized.

## Background
RELATED APPLICATION
This application is a divisional of U.S. Ser. No. 08/984,178, FILED Dec. 3, 1997, now abandoned, which is a continuation of U.S. Ser. No. 08/287,669, filed Aug. 9, 1994, now abandoned, which is a divisional of U.S. Ser. No. 07/979,638, filed Nov. 20, 1992, now abandoned, which is a continuation-in-part of U.S. Ser. No. 07/897,788 now abandoned, entitled “Cloning, Sequencing and Characterization of Two Cell Death Genes and Uses Therefor” by H. Robert Horvitz, Junying Yuan, and Shai Shaham, filed Jun. 12, 1992. The teachings of U.S. Ser. No. 07/897,788 are incorporated by reference.


GOVERNMENT FUNDING
Work described herein was supported by grants GM24663 and GM24943 from the U.S. Public Health Service. The U.S. Government has certain rights in the invention.


BACKGROUND
Cell death is a fundamental aspect of animal development. Many cells die during the normal development of both vertebrates (Glucksmann, Biol. Rev. Cambridge Philos. Soc. 26:59-86 (1951)) and invertebrates (Truman, Ann. Rev. Neurosci. 7:171-188 (1984)). These deaths appear to function in morphogenesis, metamorphosis and tissue homeostasis, as well as in the generation of neuronal specificity and sexual dimorphism (reviewed by Ellis et al., Ann. Rev. Cell Biol. 7:663-698 (1991)). An understanding of the mechanisms that cause cells to die and that specify which cells are to live and which cells are to die is essential for an understanding of animal development.
The nematode Caenorhabditis elegans is an appropriate organism for analyzing naturally-occurring or programmed cell death (Horvitz et al., Neurosci. Comment. 1:56-65 (1982)). The generation of the 959 somatic cells of the adult C. elegans hermaphrodite is accompanied by the generation and subsequent deaths of an additional 131 cells (Sulston and Horvitz, Dev. Biol. 82:110-156 (1977); Sulston et al., Dev. Biol. 100:64-119 (1982)). The morphology of cells undergoing programmed cell death in C. elegans has been described at both the light and electron microscopic levels (Sulston and Horvitz, Dev. Biol. 82:100-156 (1977); Robertson and Thomson, J. Embryol. Exp. Morph. 67:89-10 100 (1982)).
Many genes that affect C. elegans programmed cell death have been identified (reviewed by Ellis et al., Ann. Rev. Cell Biol. 7:663-698 (1991)). The activities of two of these genes, ced-3 and ced-4, are required for the onset of almost all C. elegans programmed cell deaths (Ellis and Horvitz, Cell 44:817-829 (1986)). When the activity of either ced-3 or ced-4 is eliminated, cells that would normally die instead survive and can differentiate into recognizable cell types and even function (Ellis and Horvitz, Cell 44:817-829 (1986); Avery and Horvitz, Cell 51:1071-1078 (1987); White et al., Phil. Trans. R. Soc. Lond. B. 331:263-271 (1991)). Genetic mosaic analyses have indicated that the ced-3 and ced-4 genes most likely act in a cell autonomous manner within dying cells, suggesting that the products of these genes are expressed within dying cells and either are cytotoxic molecules or control the activities of cytotoxic molecules (Yuan and Horvitz, Dev. Biol. 138:33-41 (1990)).
SUMMARY OF THE INVENTION
This invention relates to genes shown to be essential for programmed cell death, referred to herein as cell death genes, to their encoded products (RNA and polypeptides), and to antibodies directed against the encoded polypeptides. Methods and probes for identifying and screening for other cell death genes, including those of vertebrates as well as invertebrates, and possibly, microbes and plants, are described. Agents which mimic or affect the activity of cell death genes and methods for identifying these agents are also described. Bioassays which detect the activity of cell death genes and which are useful for identifying cell death genes, for testing the effect of mutations in cell death genes, and for identifying agents which mimic or affect the activity of cell death genes are also provided. This invention further relates to methods for altering (increasing or decreasing) the activity of the cell death genes or their encoded products in cells and, thus, for altering the proliferative capacity or longevity of a cell population or organism.
Specifically, the ced-3 and ced-4 genes of the nematode C. elegans have been identified, sequenced, and characterized. These genes have been shown to be required for almost all the programmed cell deaths which occur during development in C. elegans. Thus, two cell death genes and their encoded products (RNA, polypeptide) are now available for a variety of uses.
As described herein, the ced-3 and ced-4 genes can be used to identify structurally related genes from a variety of sources. Some of these related genes are likely to also function as cell death genes. Structural comparison of related cell death genes, as well as mutational analysis, can provide insights into functionally important regions or features of call death genes and gene products. This information is useful in the design of agents which mimic or which alter the activity of cell death genes.
This invention further provides methods and agents for altering (increasing or decreasing) the occurrence of cell death in a cell population or organism. Methods and agents, described herein, which decrease cell death are potentially useful for treatment (therapeutic and preventive) of disorders and conditions characterized by cell deaths, including myocardial infarction, stroke, traumatic brain injury, degenerative diseases (e.g., Huntington's disease, amyotrophic lateral sclerosis, Alzheimer's disease, Parkinson's disease, and Duchenne's muscular dystrophy), viral and other types of pathogenic infection (e.g., human immunodeficiency virus, HIV), aging and hair loss. Methods and agents which increase cell death are also provided and are potentially useful for reducing the proliferation or size of cell populations, such as cancerous cells, cells infected with viruses (e.g., HIV) or other infectious agents, cells which produce autoreactive antibodies and hair follicle cells. Such methods and agents may also be used to incapacitate or kill undesired organisms, such as pests, parasites, and recombinant organisms.



BRIEF DESCRIPTION OF THE DRAWINGS
FIG. 1 shows the genomic organization and nucleotide sequence (Seq. ID #1) of ced-4 and deduced amino acid sequence (Seq. ID #2). The genomic sequence of the ced-4 region was obtained from plasmid C10D8-5, which rescues the ced-4 mutant phenotype. Two likely transcriptional start sites are marked with downward arrows. The start of the cDNA is marked with a solid arrowhead. The positions of eight ced-4 mutations are indicated by upward arrows. Numbers on the sides indicate nucleotide positions, beginning at the start of C10D8-5. Numbers under the amino acid sequence indicate codon positions. Vertical lines between nucleotides indicate splice junctions.
FIG. 2 shows the genomic structure of the ced-4 gene and positions of ced-4 mutations. The sizes of exons and introns are indicated in base pairs (bp). The downward arrows indicate the positions of the Tc4 insertion in the ced-4 (n1416) mutant and of eight EMS-induced mutations of ced-4. The arrow pointing right indicates the direction of transcription. The solid arrowhead indicates the translation initiation site. The open arrowhead indicates the ochre termination codon.
FIG. 3 shows the sequence similarities between the Ced-4 protein and some calcium-binding proteins. The consensus sequence of the calcium-binding loop is shown at the top. The positions indicated by X, Y, Z, −X, and −Z correspond to vertices of an octahedron. The numbers above the X, Y, Z, −X and −Z correspond to the positions of the residues within the 29 amino acid EF-hand sequence. Amino acids are indicated by the single letter code. O, amino acid with an oxygen containing side chain. *, non-conserved amino acid. Position Y, Z, and −X can be any amino acid with oxygen-containing side chains. Position X is usually aspartic acid, and position −z is usually glutamic acid. Conserved amino acids are shown in bold-face. Deviations from the EF-hand consensus are underlined. The EF-hand sequences listed correspond to the following SEQ ID NO.s: ced-4 sequence 1 (SEQ ID NO.:30); ced-4 sequence 2 (SEQ ID NO.:31); Parvalbumin (carp) (SEQ ID NO.:3), (hake) (SEQ ID NO.:4), (ray) (SEQ ID NO.:5); SCBP (SEQ ID NO.:6), ICaBP (bovine first and second sequence) (SEQ ID NO.s:7 and 8, respectively; Troponin C (first through fourth sequences) (SEQ ID NO.s:9-12, respectively; Calmodulin (SEQ ID NO.:13); Trypsinogen (SEQ ID NO.:14), Fibrinogen (SEQ ID NO.:15); Villin (SEQ ID NO.:16); and GBP (SEQ ID NO.:17).
FIG. 4 shows the nucleotide sequence (Seq. ID #18) of ced-3 and deduced amino acid sequence (Seq. ID #19). The genomic sequence of the ced-3 region was obtained from plasmid pJ107, which rescues the ced-3 mutant phenotype. The likely translation initiation site is indicated by a solid arrowhead. The SL1 splice acceptor of the RNA is boxed. The positions of 12 ced-3 mutations are indicated. Repetitive elements in the introns are indicated as arrows above the relevant sequence. Numbers on the sides indicate nucleotide positions, beginning with the start of pJ107. Numbers under the amino acid sequence indicate codon positions.
FIG. 5A shows the genomic structure of the ced-3 gene and the location of the mutations. The sizes of the introns and exons are given in bp. The downward arrows indicate the positions of 12 EMS-induced mutations of ced-3. The arrow pointing right indicates the direction of transcription. The solid arrowhead indicates the translation initiation site. The open arrowhead indicates the termination codon.
FIG. 5B shows the locations of the mutations relative to the exons (numbered 1-8) and the encoded serine-rich region.
FIG. 6 is a Kyte-Doolittle hydrophobicity plot of the Ced-3 protein.
FIG. 7 shows a comparison of the Ced-3 proteins of C. elegans (line 1) (SEQ ID NO.:19) and related nematodes, C. briggsae (line 2) (SEQ ID NO.:20) and C. vulgaris (line 3) (SEQ ID NO.21). The conserved amino acids are indicated by “.”. Gaps inserted in the sequence for the purpose of alignment are indicated by “_”.
FIG. 8 shows a restriction site map of the ced-4 region and the relative positions of plasmid C10D8-5, plasmid insert pn1416, and three transcripts encoded by the region.
FIG. 9 shows physical and genetic maps of the ced-3 region on chromosome IV.
FIG. 10 summarizes experiments to localize ced-3 within C48D1. Restriction sites of plasmid C48D1 and subclone plasmids are shown. ced-3 activity was scored as the number of cell corpses in the head of L1 young animals. ++, the number of cell corpses above 10. +, the number of cell corpses below 10 but above 2. −, the number of cell corpses below 2.



DETAILED DESCRIPTION OF THE INVENTION
The ced-3 and ced-4 genes of C. elegans have been shown to be required for almost all programmed cell deaths in C. elegans development (Ellis and Horvitz, Cell 44:817-829 (1986)). The present work describes the cloning, sequencing and characterization of these genes. As a result of this work, two genes whose activities are required for cell death, referred to herein as cell death genes, and their encoded products (RNA, polypeptide) are available for a variety of uses. Described below are the cloning and characterization of the C. elegans ced-4 and ced-3 genes, methods and probes for identifying structurally related genes, methods for identifying cell death genes from a variety of organisms, methods for identifying agents which mimic or which affect the activity of cell death genes, and methods and agents for altering cell death activity and thus, for altering the occurrence of cell death in a cell population or organism.
The activity of a cell death gene is intended to include the activity of the gene itself and of the encoded products of the gene. Thus, agents and mutations which affect the activity of a gene include those which affect the expression as well as the function of the encoded RNA and protein. The agents may interact with the gene or with the RNA or protein encoded by the gene, or may exert their effect more indirectly.
The ced-4 Gene
The cloning, sequencing and characterization of the C. elegans ced-4 gene are described in Example 1. Genomic clones were obtained from a ced-4 mutant allele. generated by transposon tagging. A subclone containing as little as 4.4 kb of wild-type genomic DNA was shown to complement the ced-4 mutant phenotype (see Table 1; tables are located at the end of the Detailed Description).
A 2.2 kb mRNA was identified as the ced-4 transcript. The transcript was shown to be present at normal levels in a ced-3 mutant, suggesting that ced-3 is not a transcriptional regulator of ced-4 gene expression. Furthermore, the 2.2 kb transcript was shown to be expressed primarily during embryogenesis. This is consistent with the observation that 113 of the 131 programmed cell deaths in C. elegans are embryonic (Sulston and Horvitz, Dev. Biol. 82:110-156 (1977);
Sulston et al., Dev. Biol. 100:64-119 (1983)).
cDNA clones were further obtained and sequenced. Analysis of the cDNA and its encoded product indicates that the putative Ced-4 protein is 549 amino acids in length (FIG. 1; Seq. ID #2) and about 62,877 in relative molecular mass. The Ced-4 protein is highly hydrophilic, with a predicted pI of 5.12; there are no obvious transmembrane regions. The longest hydrophobic region is a segment of 12 amino acids from residues 382 to 393.
Sequence analysis of the ced-4 genomic clone and comparison with the cDNA sequence revealed that the ced-4 gene contains 7 introns with sizes ranging from 44 bp to 557 bp (FIG. 2).
The nucleotide sequences of eight EMS-induced ced-4 mutations were also determined. Of the eight mutations, one results in a single amino acid substitution and the other seven appear to prevent either ced-4 RNA splicing or completion of Ced-4 protein synthesis (FIG. 2 and Table 2). These seven mutations establish the null phenotype of the ced-4 gene, confirming that ced-4 function is not essential for viability.
Two regions of the inferred Ced-4 protein have sequence similarity to known calcium-binding domains (Kretsinger, Cold Spring Harbor Symp. Quant. Biol. 52:499-510 (1987)), suggesting that Ced-4 activity and hence, programmed cell death may be modulated by calcium (see FIG. 3 and Example 1). Calcium has been implicated as an essential mediator of cell death in other organisms under a variety of conditions. For example, extracellular calcium is required for glucocorticoid-induced thymocyte death (Cohen and Duke, J. Immunol. 132:38-42 (1984)), for the deaths of adult rat hepatocytes induced by certain toxins in vitro (Schanne et al., Science 206:700-702 (1979)), for agonist-induced muscle degeneration in mice (Leonard and Salpeter, J. Cell Biol. 82:811-819 (1979)) and for neuronal cell death caused by oxygen deprivation or excitotoxicity (Coyle et al., Neurosci. Res. Prog. Bull. 19:331-427 (1981); Choi, J. Neurosci. 7:369-379 (1987), Choi, Trends Neurosci. 11:465-469 (1988)). It is possible that programmed cell death is initiated during C. elegans development by an increase in intracellular calcium, which activates the Ced-4 protein to become cytotoxic. On the other hand, certain cells seem to be protected against cell death by calcium (e.g., Koike et al., Proc. Natl. Acad. Sci. USA 86:6421-6425 (1989); Collins et al., J. Neurosci. 11:2582-2587 (1991)), suggesting that increases in intracellular calcium levels may inhibit the activity of the Ced-4 protein and thereby prevent programmed cell death.
The level of the ced-4 transcript in eggs is about 20% that of the actin 1 transcript, which is relatively. abundant (Edwards and Wood, Dev. Biol. 97:375-390 (1983)). This level seems higher than might be expected if ced-4 were expressed only in dying cells, since in an embryo there are usually no more than two or three cells dying at the same time. These considerations suggest that ced-4 might be transcribed not only in dying cells but in other cells as well. Perhaps Ced-4 activity, at least during embryonic development, is regulated at a post-transcriptional level. For example, the Ced-4 protein might have to interact with other proteins or other factors (such as calcium) to cause cell death. Since the ced-3 gene is also essential for programmed cell death in C. elegans, one possibility is that the activity of the Ced-4 protein is dependent upon ced-3 function.
The ced-3 Gene
The cloning, sequencing and characterization of the ced-3 gene are described in Example 2. The ced-3 gene was cloned by mapping DNA restriction fragment length polymorphisms (RFLPs) and chromosome walking. A 7.5 kb fragment of genomic DNA was shown to complement ced-3 mutant phenotypes. A 2.8 kb transcript was further identified. The ced-3 transcript was found to be most abundant in embryos, but was also detected in larvae and young adults, suggesting that ced-3 is not only expressed in cells undergoing programmed cell death.
A 2.5 kb cDNA corresponding to the ced-3 mRNA was sequenced. The genomic sequence was also determined (FIG. 4; Seq. ID #18) and a comparison with the cDNA sequence revealed that the ced-3 gene has 8 introns which range in size from 54 to 1195 bp (FIG. 5A). The four largest introns as well as sequences 5′ of the start codon contain repetitive elements, some of which have been previously characterized in non-coding regions of other C. elegans genes such as fem-1 (Spence et al., Cell 60:981-990 (1990)), lin-12 (J. Yochem, personnal communication), and myoD (Krause et al., Cell 63:907-919 (1990)). The transcriptional start site was also mapped, and the ced-3 transcript was found to be trans-spliced to a C. elegans splice leader, SL1.
Twelve EMS-induced ced-3 alleles were also sequenced. Eight of the mutations are missense mutations, two are nonsense mutations, and two are putative splicing mutations (Table 3). The molecular nature of these mutations, together with results of genetic and developmental analyses of nematodes homozygous for these mutations, indicate that, like ced-4, ced-3 function is not essential to viability. In addition, 10 out of the 12 mutations are clustered in the C-terminal region of the gene (FIG. 5B), suggesting that this portion of the encoded protein may be important for activity.
The ced-3 gene encodes a putative protein of 503 amino acids (FIG. 4; Seq. ID #19). The protein is very hydrophilic and no significantly hydrophobic region can be found that might be a transmembrane domain (FIG. 6). One region of the ced-3 protein is very rich in serine. Sequence comparison of two additional ced-3 genes from related nematodes, C. briggsae and C. vulgaris, suggests that the exact sequence in this serine-rich region may not be important but that the serine-rich feature is (FIG. 7; Seg. ID #19-21). This hypothesis is supported by the analysis of ced-3 mutations: none of 12 EMS-induced ced-3 mutations is in the serine-rich region (FIG. 5B).
The conservation of the serine-rich feature among the ced-3 genes of different nematodes suggests that the serine-rich region may act in semi-specific protein-protein interactions, similar to acid blobs in transcription factors and basic residues in nuclear localization signals. In all these cases, the exact primary sequence is not important.
It is possible that the serine residues in the Ced-3 and Ced-4 proteins may be targets for a Ser/Thr kinase, and that the activity of these proteins may be regulated post-translationally by protein phosphorylation. McConkey et al. (J. Immunol., 145:1227-1230 (1990)) have shown that phorbol esters, which stimulate protein kinase C, can block the death of cultured thymocytes induced by exposure to Ca++ ionophores or glucocorticoids (Wyllie, Nature 284:555-556 (1980); Wyllie et al., J. Path. 142:67-77 (1984)). It is possible that protein kinase C may inactivate certain cell death proteins by phosphorylation, and thus, inhibit cell death and promote cell proliferation. Several agents that can elevate cytosolic cAMP levels have been shown to induce thymocyte death, suggesting that protein kinase A may also play a role in mediating thymocyte death. Further evidence suggests that abnormal phosphorylation may play a role in the pathogenesis of certain cell-degenerative diseases. For example, abnormal phosphorylation of the microtubule-associated protein Tau is found in the brains of Alzheimer's disease and Down's syndrome patients (Grundke-Iqbal et al., Proc. Natl. Acad. Sci. USA 83:4913-4917 (1986); Flament et al., Brain Res. 516:15-19 (1990)). Thus, it is possible that phosphorylation may have a role in regulating programmed cell death in C. elegans. This is consistent with the fairly high levels of ced-3 and ced-4 transcripts which suggest that transcription regulation alone may be insufficient to regulate programmed cell death.
Structurally and Functionally Related Genes
As a result of the work described herein, it is possible to identify genes which are structurally and/or functionally related to ced-3 or ced-4. Such genes are expected to be found in a variety of organisms, including vertebrates (e.g., mammals and particularly humans), invertebrates (e.g., insects), microbes (e.g., yeast) and possibly plants. Structurally related genes refer herein to genes which have some structural similarity to the nucleotide sequences (genomic or cDNA) of one or both of the ced-3 or ced-4 genes, or whose encoded proteins have some similarity to one or both of the amino acid sequences of the Ced-3 or Ced-4 proteins. Functionally related genes refer to genes which have similar activity to that of ced-3 and ced-4 in that they cause cell death. Such genes can be identified by their ability to complement ced-3 or ced-4 mutations in bioassays, as described below.
Previous studies are consistent with the hypothesis that genes similar to the C. elegans ced-3 and ced-4 genes may be involved in the cell deaths that occur in both vertebrates and invertebrates. Some vertebrate cell deaths share certain characteristics with the programmed cell deaths in C. elegans that are controlled by ced-3 and ced-4. For example, up to 14% of the neurons in the chick dorsal root ganglia die immediately after their births, before any signs of differentiation (Carr and Simpson, Dev. Brain Res. 2:57-162 (1982)). Genes like ced-3 and ced-4 could well function in this class of vertebrate cell death. In addition, genes related to ced-3 and ced-4 could function in many other types of vertebrate cell death processes, including those involving cells that die long after their births and those that die as a result of stress (e.g., oxygen deprivation) or disease.
Genetic mosaic analysis has suggested that the ced-3 and ced-4 genes act within cells that undergo programmed cell death, rather than through cell-cell interactions or diffusible factors (Yuan and Horvitz, Dev. Biol. 138:33-41 (1990)). Many cell deaths in vertebrates seem different in that they appear to be controlled. by interactions with target tissues. For example, it is thought that a deprivation of target-derived growth factors is responsible for vertebrate neuronal cell deaths (Hamburger and Oppenheim, Neurosci. Comment. 1:39-55 (1982)); Thoenen et al., in: Selective Neuronal Death, Wiley, N.Y., 1987, Vol. 126, pp. 82-85). However, even this class of cell death could involve genes like ced-3 and ced-4, since pathways of cell death involving similar genes and mechanisms might be triggered in a variety of ways. Supporting this idea are several in vitro and in vivo studies which show that the deaths of vertebrate as well as invertebrate cells can be prevented by inhibitors of RNA and protein synthesis, suggesting that activation of genes is required for these cell deaths (Martin et al., J. Cell Biol. 106:829-844 (1988); Cohen and Duke, J. Immunol. 132:38-42 (1984); Oppenheim and Prevette, Neurosci. Abstr. 14:368 (1988); Stanisic et al., Invest. Urol. 16:19-22 (1978); Oppenheim et al., Dev. Biol. 138:104-113 (1990); Fahrbach and Truman, in: Selective Neuronal Death, Ciba Foundation Symposium, 1987, No. 126, pp. 65-81). It is possible that the genes induced in these dying vertebrate and invertebrate cells are cell death genes similar to the C. elegans genes ced-3 and ced-4.
Also supporting the hypothesis that cell death in C. elegans is mechanistically similar to cell death in vertebrates is the observation that the protein product of the C. elegans gene ced-9 is similar in sequence to the human protein Bcl-2. ced-9 has been shown to prevent calls from undergoing programmed cell death during nematode development by antagonizing the activities of ced-3 and ced-4 (Hengartner, et al., Nature 356:494-499 (1992)). The bcl-2 gene has also been implicated in protecting cells against cell death. It seems likely that the genes and proteins with which ced-9 and bcl-2 interact are similar as well.
Genes which are structurally related to ced-3 or ced-4 are likely to also act as cell death genes. Structurally, related genes can be identified by any number of detection methods which utilize a defined nucleotide or amino acid sequence or antibodies as probes. For example, nucleic acid (DNA or RNA) containing all or part of the ced-3 or ced-4 gene can be used as hybridization probes or as polymerase chain reaction (PCR) primers. Degenerate oligonucleotides derived from the amino acid sequence of the Ced-3 or Ced-4 proteins can also be used. Nucleic acid probes can also be based on the consensus sequences of conserved regions of genes or their protein products. In addition, antibodies, both polyclonal and monoclonal, can be raised against the Ced-3 and/or Ced-4 proteins and used as immunoprobes to screen expression libraries of genes.
One strategy for detecting structurally related genes in other organisms is to initially probe animals which are taxonomically closely related to the source of the probes, for example, probing other worms with a ced-3 or ced-4 probe. Closely related species are more likely to possess related genes or gene products which are detected with the probe than more distantly related organisms. Sequences conserved between ced-3 or ced-4 and these new genes can then be used to identify similar genes from less closely related species. Furthermore, these new genes provide additional sequences with which to probe the molecules of other animals, some of which may share conserved regions with the new genes or gene products but not with ced-3, ced-4, or their gene products. This strategy of using structurally related genes in taxonomically closer organisms as stepping stones to genes in more distantly related organisms can be referred to as walking along the taxonomic tree.
Groups of structurally related genes, such as those obtained by using the above-described strategy, can be referred to as gene families. Comparison of members within a gene family, or their encoded products,.may indicate functionally important features of the genes or their gene products. Those features which are conserved are likely to be significant for activity. Such conserved sequences can then be used both to identify new members of the gene family and in drug design and screening. For example, as described in Example 2, genes similar to ced-3 from two other species of nematodes (C. briggsae and C. vulgaris) were identified and characterized. Serine-rich regions were found in the polypeptides encoded by all three genes. Although the sequence of the serine-rich region was not well conserved, the number of serines was conserved, suggesting that the serine-rich feature, but not the exact sequence of the serine-rich region, is significant for function.
Functionally important regions can also be identified by mutagenesis. For example, inactivating mutations of ced-3 were found to cluster within a region near the COOH-terminus (FIG. 5B), suggesting that this region is a functionally important domain of the Ced-3 protein. Further mutational analyses can be carried out on the ced-3 and ced-4 genes; mutants with novel properties, as well as other regions important for activity, may be discovered. Mutations and other alterations can be accomplished using known methods, such as in vivo and in vitro mutagenesis (see, e.g., Ausubel et al. (eds.), Current Protocols in Molecular Biology, Greene Publishing Associates and Wiley-Interscience, New York).
Bioassays and Agents Which Affect the Activity of Cell Death Genes
This invention further provides bioassays which detect the activity of cell death genes. The bioassays can be used to identify novel cell death genes, to identify mutations which affect the activity of cell death genes, to identify genes which are functionally related to known cell death genes, such as ced-3 or ced-4, to identify genes which interact with cell death genes, and to identify agents which mimic or affect the activity of cell death genes (e.g., agonists and antagonists). For example, the bioassays can be used to screen expression gene libraries for cell death genes from other organisms.
In this bioassay, genes or agents are introduced into nematodes to test their effect on cell deaths in vivo. Wild-type, mutant, and transgenic nematodes can be used as appropriate for the effect being tested. In one embodiment of this bioassay, transgenic nematodes are produced using a candidate cell death gene, a mutant cell death gene, or genes from an expression library, to observe the effect of the transgene on the pattern of programmed cell deaths during development of the nematode. For example, a gene which is structurally related to ced-3 can be used to produce a transgenic animal from a mutant nematode which underexpresses or expresses an inactivated ced-3 gene to see if the related gene can complement the ced-3 mutation and is thus, functionally as well as structurally related to ced-3. cDNA or genomic libraries can be screened for genes having cell death activity. Genes which interact with cell death genes to enhance or suppress their activity can also be identified by this method.
In another embodiment of the bioassay, wild-type, mutant, or transgenic nematodes are exposed to or administered peptides and other molecules in order to identify agents that mimic, increase, or decrease the activity of a cell death gene. For example, wild-type animals can be used to test agents that inactivate or antagonize the activity of ced-3 or ced-4 and hence, decrease cell deaths, or that activate or enhance ced-3 or ced-4 activity and increase cell deaths. Mutant animals in which ced-3 or ced-4 is inactivated can be used to identify agents or genes which mimic ced-3 or ced-4 in causing cell deaths. Mutant animals in which ced-3 or ced-4 is overexpressed or constitutively activated can similarly be used to identify agents that prevent ced-3 or ced-4 from causing cell death. Transgenic animals in which a wild-type or mutant form of an exogenous cell death gene causes excess cell deaths due to overexpression or hyperactivity can be used to identify agents that inactivate or inhibit the activity of the transgene. Similarly, transgenic animals in which a wild-type or mutant form of an exogenous cell death gene is underexpressed or inactive can be used to identify agents that activate or increase its activity. Test molecules can be introduced into nematodes by microinjection, diffusion, ingestion, shooting with a particle gun, or other method.
Mutated cell death genes with novel properties may be identified by the above bioassay. For example, constitutively activated or hyperactive cell death genes may be isolated which may be useful as agents to increase cell deaths. Mutations may also produce genes which do not cause cell death but which antagonize the activity of the wild-type gene.
Agents can be obtained from traditional sources, such as extracts (e.g., bacterial, fungal or plant) and compound libraries, or by newer methods of rationale drug design. Information on functionally important regions of the genes or gene products, gained by sequence and/or mutational analysis, as described above, may provide a basis for drug design. The activity of the agents can be verified both by in vivo bioassays using nematodes which express various forms of ced-3, ced-4, or related genes, as described above, and by in vitro systems, in which the genes are expressed in cultured cells, or in which isolated or synthetic gene products are tested directly in biochemical experiments. The agents may include all or portions of the ced-3, ced-4, or related genes, mutated genes, and all or portions of the gene products (RNA, including antisense RNA, and protein), as well as nucleic acid or protein derivatives, such as oligonucelotides and peptides, peptide and non-peptide mimetics, and agonists and antagonists which affect the activity or expression of the cell death genes. The acents can also be portions or derivatives of genes or gene products which are not cell death genes but which regulate the expression of, interact with, or otherwise affect the function of cell death genes or gene products.
Uses of the Invention
Using the above-described probes and bioassays, the identification and expression of ced-3, ced-4 or related cell death genes in cultured cells, tissues, and whole organisms can be studied to gain insights into their role in development and pathology in various organisms. For example, the detection of abnormalities in the sequence, expression, or activity of a cell death gene or gene product may provide a useful diagnostic for diseases involving cell deaths.
This invention further provides means of altering or controlling the activity of a cell death gene in a cell, and, thus, affecting the occurrence of cell death. Activity of the cell death gene can be altered to either increase or decrease cell deaths in a population of cells and, thus, affect the proliferative capacity or longevity of a cell population, organ, or entire organism.
Agents which act as inactivators or antagonists of the activity of ced-3, ced-4, or other cell death genes can be used to prevent or decrease cell deaths. Such agents are useful for treating (i.e., for both preventive and therapeutic purposes) disorders and conditions characterized by cell deaths, including neural and muscular degenerative diseases, stroke, traumatic brain injury, myocardial infarction, viral (e.g., HIV) and other types of pathogenic infections, as well as cell death associated with normal aging and hair loss. The agent can be delivered to the affected cells by various methods appropriate for the cells or organs being treated, including gene therapy. For example, anti-sense RNA encoded by all or a part of a cell death gene which is complementary to the mRNA can be delivered to a population of cells by an appropriate vector, such as a retroviral or adenoviral vector, or an antagonist of cell death activity can be infused into a wound area to limit tissue damage.
Methods and agents which cause or increase cell deaths are also useful, for example, for treating disorders characterized by an abnormally low rate or number of cell deaths or by excessive cell growth, such as neoplastic and other cancerous growth. Such methods and agents are also useful for controlling or eliminating cell populations, such as cells infected with viruses (e.g., HIV) or other infectious agents, cells producing autoreactive antibodies, and hair follicle cells. in addition, methods and agents which increase cell death can be used to kill or incapacitate undesired organisms, such as pests, parasites and genetically engineered organisms. All or portions of ced-3, ced-4, or related cell death genes, active mutant genes, their encoded products, agents which mimic the activity of cell death genes, and activators and agonists of cell death genes can be used for this purpose.
For example, cell death genes can be used to kill cells infected with the human immunodeficiency virus (HIV), and thus, prevent or limit HIV infection in an individual. A recombinant gene can be constructed, in which a cell death gene is under the control of a viral promoter which is specifically activated by a viral protein; the recombinant gene is introduced into HIV infected cells. HIV-infected cells containing the viral activator protein would express the cell death gene product and be killed, and uninfected cells would be unaffected.
Alternatively, an antagonist of ced-3 or ced-4 activity (such as antisense RNA) can be expressed under the control of a viral-specific promoter and in this way, be used to prevent the cell death associated with viral (e.g., HIV) infection.
In another example, cell death genes can be used as suicide genes for biological containment purposes. Genetic engineering of suicide genes into recombinant organisms has been reported in bacteria (Genetic Engineering News, November 1991, p. 13): suicide genes were engineered to be expressed simultaneously with the desired recombinant gene product so that the recombinant bacteria die upon completion of their task. The present invention provides suicide genes which are useful in a variety of organisms in addition to bacteria, for example in insects, fungi, and transgenic rodents. Suicide genes can be constructed by placing the coding sequence of an exogenous cell death gene or an agonist of an endogenous cell death gene of the organism in an expression vector suitable for the organism.
In addition, agents which increase cell death are useful as pesticides (e.g., anthelminthics, nematicides). For example, many nematodes are human, animal, or plant parasites. ced-3, ced-4, or other nematode cell death genes, their gene products, mimetics, and agonists can be used to reduce the nematode population in an area, as well as to treat individuals already infected with the parasite or protect individuals from infection. A transgenic plant or animal carrying a constitutively activated ced-3 gene, ced-4 gene, or other cell death gene specific to nematodes can be protected from nematode infection in this way.
The subject invention will now be illustrated by the following examples, which are not intended to be limiting in any way.2
EXAMPLE 1
CLONING, SEQUENCING AND CHARACTERIZATION OF THE CED-4 GENE
MATERIALS AND METHODS
General Methods and Strains
Techniques used for the culturing of C. elegans were essentially as described by Brenner (Genetics 77:71-94 (1974)). All strains were grown at 20° C. DNA was prepared from worms grown on Petri dishes containing agarose seeded with E. coli strain HB101. RNA was prepared from mass cultures grown in liquid. Usually, the bacterial pellet from a 2 L overnight culture of E. coli HB101 grown in superbroth (12 g Bacto-tryptone, 24 g yeast extract, 8 ml 50% glycerol, 900 ml H2O; after autoclaving, 100 ml 0.17 M KH2HPO4 and 0.72 K2HPO4 were added) was resuspended in 500 ml S basal medium (Brenner, 1974 supra), and worms were added from one or two 10 cm Petri dishes in which the bacterial lawns had just been consumed. Worms were harvested about 4-5 days later by centrifugation and washed in M9 buffer (Brenner, 1974 supra). The yield was about 5-10 ml of packed worms.
Nomarski differential interference contrast microscopy was used to examine individual cells in living nematodes (Sulston and Horvitz, Dev. Biol. 82:110-156 (1977)). Methods for scoring the Cad phenotype of ced-1, ced-4 and ced-1; ced-4 double mutants have been described by Ellis and Horvitz, (Cell 44:817-829 (1986)) and by Yuan and Horvitz, (Dev. Biol. 138:33-41 (1990)).
The wild-type parent of all mutant strains used in these experiments was C. elegans variety Bristol strain N2 (Brenner, 1974 supra). The genetic markers used are listed below. These markers have been described (Brenner, 1974 supra; Hodgkin et al., in: The Nematode Caenorhabditis elegans, Wood and the Community of C. elegans Researchers (eds.), Cold Spring Harbor Laboratory, New York, 1988, pp. 491-584; Finney et al., Cell 55:757-769 (1988)). The strain TR679 carries the mutator mut-2(r459) (Collins et al., Nature 328:726-728 (1987)). The ced-4 alleles n1894, n1920, n1947, n1948, n2247, and n2273 were characterized in the present work. Genetic nomenclature follows the standard system for C. elegans (Horvitz et al., Mol. Gen. Genet. 275:129-133 (1979)):

    
    
        LG I: ced-1(e1735), unc-54(r323)
        LG III: unc-86(n1351), ced-4(n1162, n1416, n1894, n1920, n1947, n1948, n2247, n2273, n1416 n1712, n1416 n1713), unc-79(e1068), dpy-17 (e164)
        LG IV: unc-31(e928), ced-3(n717)
        LG V: egl-1(n986), unc-76(e911)

Genomic Libraries

    
    


A 4-6 kb size-selected phage library was constructed from ced-4(n1416) DNA as follows. Genomic DNA was digested with HindIII and run on a low-melting agarose gel. DNA migrating within the 4-6 kb size range was excised, and the low-melting agarose was removed by phenol extraction and precipitation (Maniatis et al., Molecular Cloning: A Laboratory Manual, Cold Spring Harbor Laboratory (1983)). These DNA fragments were ligated to HindIII-digested DNA from phage λNM1149 (Murray, Phage Lambda and Molecular Cloning, Cold Spring Harbor Laboratory, 1983, pp. 395-432). The product DNA was packaged with packaging extract from Promega. This library had a total of 140,000 plaque-forming units (pfu), of which 70% were recombinants, as estimated from the ratio of pfu on bacteria C600hfl and C600.
The phage genomic library (provided by J. Sulston). was prepared by partial digestion of wild-type C. elegans genomic DNA with Sau3A and cloning into the BamHI site of phage vector λ2001 (Karn et al., Gene 32:217-224 (1984)).
Tc4 Probe
The Tc4 probe used for cloning the ced-4 gene and for Southern blots was Tc4-n1351, which contains a Tc4 element isolated from an unc-86(n1351) mutant strain (Finney et al., Cell 55:757-769 (1988); Yuan et al., Proc. Natl. Acad. Sci. USA 88:3334-3338 (1991)). DNA was labelled with 32P using either the nick-translation procedure described by Maniatis et al. (1983 supra) or the oligo-labelling procedure described by Feinberg and Vogelstein (Anal. Biochem, 132:6-13 (1983)).
RNA Preparation, Northern Blot and Primer Extension
Total C. elegans RNA was extracted using guanidine isothiocyanate (Kim and Horvitz, Genes & Dev. 4:357-371 (1990)). Poly(A)+ RNA was selected from total RNA by a poly(dT)-column (Maniatis et al., 1983 supra). To prepare stage-synchronized animals, eggs were obtained from gravid C. elegans adults grown at 20° C. in liquid culture. A 5-10 ml sample of animals was treated with 50 ml of NaOCl/NaOH solution (10 ml NaOCl, 1 g NaOH, 40 ml H2O) for about 10 minutes with vortexing until the adults were dissolved. Eggs were centrifuged and washed three times with M9 buffer. Isolated eggs were allowed to hatch in S basal medium without food for 14 hours at 20° C. with shaking. L1 larvae were collected by low-speed centrifugation after growth on E. coli HB101 for 2 hours, L2 larvae after 12 hours, L3 larvae after 24 hours, L4 larvae after 36 hours and adults after 48 hours. Northern blot analysis using DNA probes was performed essentially as described by Meyer and Casson (Genetics 106:29-44 (1986)), except that RNA was transferred from the gel to the Gene Screen filter (DuPont, Wilmington, Del.) by capillary action.
Quantitation of ced-4 expression during embryonic development was done by hybridizing two duplicate northern blots with ced-4 cDNA clone SK2-2 and with a genomic DNA clone for the actin 1 gene, pW-16-210, which hybridizes to the 3′ untranslated region of the actin 1 transcript (Krause and Hirsh, in: Molecular Biology of the Cytoskeleton, Borisy et al. (eds.), Cold Spring Harbor Laboratory, 1984, pp. 287-292). The two probes were of the same specific activity (4×108 counts/minute/μg). The emission of β particles from the ced-4 and actin 1 bands was counted using a β counter (Betagen, Waltham, Mass.). The readings were 7.7 counts/minute for the actin 1 band and 1.4 counts/minute for the ced-4 band.
The primer extension protocol was that of Sambrook et al. (Molecular Cloning: A Laboratory Manual, 2nd edition, Cold Spring Harbor Laboratory, 1989, pp. 7.79-7.83), using the primer ATTGGCGATCCTCTCGA (Seq. ID #22). To define the lengths of the reaction products, a sequencing reaction using this primer and C10D8-5 as template was run adjacent to the product of the primer extension reaction in the sequencing gel.
Direction of Transcription
The direction of transcription was determined by hybridizing northern blots with single-stranded RNA probes. The Bluescribe plasmid containing the insert pn1416 was linearized by digestion with either BamHI or HindIII, which cleaved at one or the other end of the insert. The linearized product was transcribed using T3 or T7 RNA polymerase, respectively, generating RNA from each strand. These RNA products were used to probe Northern blots according to a protocol developed by Z. Liu and V. Ambros: Filters were prehybridized in 50% formamide, 50 mM sodium phosphate (pH 6.5), 5×SSC, 8×Denhardt's, 0.5% SDS, 250 μg/ml salmon sperm DNA and then hybridized with probe at 55° C. and washed in 4×SSC, 0.1% SDS at 60° C. 3 times for 20 minutes each and then in 2×SSC, 0.1% SDS once at 60° C. for 20 minutes. Northern blot experiments showed that the single-stranded RNA probe transcribed by T3 RNA polymerase hybridized to the 2.2 kb ced-4 mRNA, while the probe made by T7 RNA polymerase did not. This result indicates that the direction of the transcription is from the BamHI site toward the HindIII site of pn1416.
Determination of DNA Sequence
For determining DNA sequences, serial deletions were made according to Henikoff (Gene 28:351-359 (1984)). DNA sequences were determined using Sequenase and protocols obtained from US Biochemicals (Cleveland, Ohio). The ced-4 DNA sequence was confirmed by sequencing both strands of cDNA and genomic DNA clones.
Cloning of the Cosmid Fragment C10D8-5
The cosmid C10D8 was digested with EcoRI. Two EcoRI fragments of 2.2 kb (r5) and 2.4 kb (r7), both of which hybridized to a mixture of ced-4 cDNA subclones SK2-1 and SK2-2, were isolated. r7, which hybridized to SK2-1, which contains the 3′ half of ced-4 cDNA clone SK2, was cloned into the EcoRI site of plasmid pBSKII (Stratagene). The EcoRI site at the 3′ end of r7 was deleted by digesting with Styl, which cut once at 0.2 kb from the 3′ end of the insert, and SalI, which cut once in the polylinker, and then religating. The deleted r7 plasmid was linearized with EcoRI and ligated with EcoRI-digested r5, which hybridized to Sk2-2, the 5′ half of ced-4 cDNA SK2. Clones were analyzed for the correct orientation of the r5 insert based on the cDNA restriction map. One such correctly oriented clone was named C10D8-5.
Microinjection and Transformation
The procedure;for microinjecting DNA into the gonad to obtain germline transformants was basically that of Fire (EMBO J. 5:2673-2680 (1986)) with modifications introduced by J. Sulston. Cosmid DNA to be injected was purified twice using CsCl-gradient centrifugation (Maniatis et al., 1983 supra). Plasmid DNA to be injected was prepared by alkaline minipreps (Maniatis et al., 1983 supra). DNA was treated with RNAase A (37° C., 30 minutes) and then with proteinase K (55° C., 30 minutes), extracted with phenol and then chloroform, precipitated twice (first in 0.3 M sodium acetate and then in 0.1 M potassium acetate, pH 7.2), and resuspended in 5 ul of injection buffer (Fire, 1986 supra). DNA concentrations used for injection were 0.1-1.0 mg/ml.
All transformation experiments used a ced-1; ced-4(n1162); unc-31 strain as the recipient. The expression of the Ced-4 phenotype was quantified by counting the number of cell corpses in the heads of young L1 animals. The cosmid C10D8 or plasmid subclones of C10D8 were mixed with cosmid C14G10, which contains the wild-type unc-31(+) gene, at a ratio of 2:1 or 3:1 to increase the likelihood that a phenotypically non-Unc transformant would contain the cosmid or plasmid being tested. Generally, 20-30 animals were injected in one experiment. Non-Unc F1 progeny of injected animals were isolated three to four days later. About 1⁄2 to 1⁄3 of the non-Unc progeny transmitted the non-Unc phenotype to their progeny and could be established as lines of transformants. Young L1 non-Unc progeny of such non-Unc transformants were examined using Nomarski optics to determine the number of cell corpses present in the heads.
Ced-4 Fusion Protein and Antibody Preparation
To express a Ced-4 fusion protein in E. coli, a clone containing both the 5′ and 3′ halves of the ced-4 cDNA (SK2-2 and SK2-1) in the expression vector pET-5a (Rosenberg et al., Gene 56:125-135 (1987)) was constructed. The fusion protein expressed by this vector was expected to include 11 amino acids of phage T7 gene 10 protein, 5 amino acids of linker and the 546 amino acids encoded by ced-4 cDNA SK2. The pJ76 plasmid, which encodes this fusion protein, was transformed into bacterial strain BL21. ced-4 fusion protein was produced by this transformed strain, as expected, and subjected to electrophoresis on a polyacrylamide gel. A band, with mobility equivalent to about 64×103 Mr, specific to the transformed strain was exercised and used to immunize three rabbits. Sera from all three rabbits tested positive on western. blots (Towbin et al., Proc. Natl. Acad. Sci. USA 76:4350-4354 (1979)). These sera were purified sing immunoblots (Harlow and Lane, Antibodies: A Laboratory Manual, Cold Spring Harbor Laboratory, 1988).
RESULTS
Cloning of the ced-4 Gene by Transposon Taggaing
The ced-4 allele n1416 in the C. elegans strain TR679 was isolated, which carries the mutator mut-2(r459) and shows an elevated frequency of transposition elements (Collins et al., Nature 328:726-728. (1987); Yuan et al., Proc. Natl. Acad. Sci. USA 88:3334-3338 (1991)). The ced-4(n1416) mutation is closely linked to a newly transposed copy of the C. elegans transposon Tc4 (Yuan et al., 1991 supra). Using Tc4 as a probe, this novel Tc4 element and its flanking region was cloned as a 5 kb HindIII fragment from a 4-6 kb size-selected ced-4(n1416) genomic phage library. A 3 kb adjacent to this Tc4 element was isolated by digesting the 5 kb HindIII fragment with BamHI. This 3 kb fragment, called pn1416, was cloned into the Bluescribe M13+ plasmid vector (Stratagene),.
When used as a probe on Southern blots, pn1416 hybridized to a 3.4 kb HindIII fragment in DNA of wild-type (strain N2) and two non-Ced revertants of ced-4(n1416), ced-4(n1416 n1712) and ced-4(n1416 n1713) (Yuan and Horvitz, Dev. Biol. 138:33-41 (1990)), and a 5 kb HindIII fragment in ced-4(n1416) animals. The hybridizing band in ced-4(n1416) DNA is 1.6 kb larger than that of the wild-type or the revertants, indicating that an insertion of this size is present in the ced-4(n1416) strain and is deleted in both revertants. These observations indicate that the Tc4 insertion in ced-4(n1416) animals is responsible for their Ced-4 mutant phenotype and suggest that pn1416 contains at least part of the ced-4 gene.
To isolate additional genomic DNA from the region of this Tc4 insertion, pn14l6 was used to probe a C. elegans Bristol N2 genomic DNA phage library. Five phage clones with inserts of 10 to 15 kb were isolated and shown to share a 3 kb BamHI-HindIII fragment that hybridized to pn1416. These phage clones were used to identify cosmids that hybridized to them and that were members of a 600 kb contig of overlapping cosmids (Coulson et al., Proc. Natl. Acad. Sci. USA 83:7821-7825 (1986)). By using the phage clones as probes to hybridize to Southern blots, a cosmid C10D8 was identified as containing all regions of genomic DNA present in all five phage clones and in pn1416.
The ced-4 Mutant Phenotype Can Be Rescued by a 4.4 kb DNA Fragment
To identify ced-4(+) DNA capable of complementing the Ced-4 mutant phenotype, the cosmid C10D8 was injected into the oocytes of ced-4(n1162) animals. To facilitate the identification of transgenic animals, a mutation in the unc-31 gene, which affects locomotion, was included as a marker for co-transformation (Kim and Horvitz, Genes & Dev. 4:357-371 (1990)). Cosmid C14G10, which contains the wild-type allele of unc-31 and does not have Ced-4-rescuing activity was coinjected with cosmid C10D8 into ced-1(e1735); unc-31(e928); ced-4(n1162) animals. The ced-1 mutation was included to facilitate the scoring of the ced-4 mutant phenotype (Ellis and Horvitz, Cell 44:817-829 (1986)). Specifically, when a cell undergoes programmed cell death in C. elegans, its corpse is quickly engulfed and destroyed by a neighboring cell (Robertson and Thomson, J. Embryol. Exp. Morph. 67:89-100 (1982); Sulston et al., Dev. Biol. 100:64-119 (1983)). A ced-1 mutation prevents this engulfment, allowing the cell corpse to remain intact (Hedgecock et al., Science 220:1277-1280: (1983)). Thus, in a first or second stage (L1 or L2) ced-1 mutant larva, many cell corpses are present and can be easily visualized using Normaski optics. ced-4 mutations prevent cell death and the appearance of these corpses. Thus, suppression of the Ced-4 mutant phenotype by a wild-type ced-4 gene can be observed and readily quantified in a ced-1 mutant background based on an increase in the number of visible cell corpses.
From one such microinjection experiment, three non-Unc animals rescued for the Unc-31 mutant phenotype were picked from among the F1 progeny, and from one of them a line of non-Unc transformants was obtained. No true-breeding non-Unc animals could be isolated from this line: about 25% of the progeny of all non-Unc animals were Unc. since no inviable zygotes were observed among the progeny of these non-Unc animals, this transformant did not carry a recessive lethal insertion mutation. Rather, it seems likely that the injected DNA was maintained as an extrachromosomal array that was segregated to only some gametes, as has been reported previously for many other C. elegans transgenic strains (e.g., Stinchcomb et al., Mol. Cell Biol. 82:110-156 (1985);. Fire, EMBO J. 5:2673-2680 (1986); Way and Chalfie, Cell 54:5-16 (1988)). This putative extrachromosomal array was named nEx1. Young L1 progeny of nEx1-containing animals were examined using Nomarski optics for the Ced-4 phenotype.
Young L1 ced-1 animals have an average of 23 cell corpses in the head, while ced-1 (e1735); ced-4 (n1162) animals have an average of 0.6 cell corpses (Ellis and Horvitz, Cell 44:817-829 (1986)). Young L1 ced-1; ced-4(n1162); nEx1 animals had an average of nine cell corpses in the head. These results indicate that cosmid C10D8 restored significant, but not total, ced-4(+) activity in the transformants.
To delineate the ced-4 gene within C10D8, various subclones of C10D8 were injected into ced-4 mutant animals and tested for their ability to rescue the Ced-4 mutant phenotype (Table 1). The smallest subclone plasmid that could rescue the ced-4 phenotype as effectively as cosmid C10D8 was a 4.4 kb fragment, called C10D8-5. C10D8-5 and the unc-31(+)-containing cosmid C14G10 were coinjected into ced-1; unc-31; ced-4(n1162) animals. Two lines of non-Unc transformants were isolated. Since these animals continued to segregate Unc animals and did not produce inviable zygotes, both appeared to carry extrachromosomal arrays, which were designated nEx7 and nEx8. Young L1 animals from these transformant strains had an average of 11.5 cell corpses in their heads, indicating that plasmid C10D8-5 restored ced-4(+) activity as well as did cosmid C10D8 (Table 1).
Identification of a ced-4 Transcript
Restriction sites of plasmid C10D8-5 (which can rescue the Ced-4 phenotype) and pn1416 (which contains sequences adjacent to the Tc4 insertion site) were mapped. C10D805 was found to overlap with 2 kb of sequence in pn1416, including the Tc4 insertion site (FIG. 8).
In Northern blot experiments, both pn1416 and C10D8-5 were used to probe poly(A)+ RNA populations of mixed developmental stages of wild-type (strain N2), ced-4(n1416), and ced-4(n1416 n1712) and ced-4(n1416 n1713) revertant animals. pn1416 hybridized to a 2.2 kb transcript and an 0.9 kb transcript in RNA from N2 animals, and a 3 kb transcript, a transcript slightly larger than the wild-type 2.2 kb transcript, and a transcript slightly smaller than the wild-type 0.9 kb transcript in ced-4(n1416) animals. The 3.8 kb RNA contained Tc4 sequence (see below), suggesting that this RNA resulted from the insertion of the 1.6 kb Tc4 sequence into the ced-4 sequence encoding 2.2 kb transcript. The transcript slightly larger than the 2.2 kb wild-type transcript did not contain Tc4 sequence. This ced-4(n1416) RNA might have been an aberrant transcript containing sequences adjacent to the ced-4 gene: when pn1416 was used as a probe, the wild-type 2.2 kb and the slightly larger transcript in this mutant were relatively similar in intensities, whereas when ced-4 cDNA clone SK2-1 was used as a probe, this mutant transcript was not detected (see below). These observations indicate that the ced-4(n1416) 2.2 kb transcript contains sequences from the ced-4 region but does not contain sequences corresponding to at least the 3′ half of the ced-4 mRNA. The two revertants of ced-4(n1416), ced-4(n1416 n1712) and ced-4(n1416 n1713), contained both 2.2 kb and 0.9 kb transcripts with similar sizes to the wild-type transcripts. Thus, both the 2.2 kb and the 0.9 kb transcripts were altered in ced-4(n1416) animals, and both were restored in the two non-Ced revertants.
To determine if any of the transcripts contains Tc4 sequence, the Northern blots were probed with Tc4-n1351, which contains the 1.6 kb Tc4 element present in the Tc4-induced mutant unc-86(n1351) as well as 4 kb of unc-86 sequences. Tc4-n1351 hybridized both to a 3.8 kb transcript of the Tc4-induced mutant ced-4(n1416) and to a 1.5 kb unc-68 transcript in both ced-4(n1416) and N2 animals.
To determine whether one or both of the 2.2 kb and 0.9 kb transcripts are encoded by ced-4, subclone C10D8-5, which rescued the Ced-4 phenotype, was used to probe the Northern blots. C10D8-5 detected the wild-type 2.2 kb transcript, the ced-4(n1416) transcript slightly larger than the 2.2 kb transcript, and the ced-4(n1416) 3.8 kb transcript. C10D8-5 did not hybridize to the 0.9, kb transcript, indicating that this transcript is unlikely to be encoded by ced-4. C10D8-5 also detected a 1.4 kb transcript, which was not altered by the Tc4 insertion in ced-4(n1416) animals only a 470 bp EcoRI-StuI fragment at one end of C10D8-5 hybridized to this 1.4 kb RNA. Since C10D8-5 did not contain the complete coding region for this RNA, and since this RNA was unaffected in ced-4(n1416) animals, this 1.4 kb RNA seems unlikely to be a ced-4 transcript. The relationships among cosmid C10D8-5, pn1416 and the 0.9 kb, 1.4 kb and 2.2 kb transcripts are summarized in FIG. 8.
On Northern blots probed with the ced-4 cDNA clone SK2-1, the level of the 2.2 kb transcript showed significant reduction in all three independently derived EMS-induced ced-4 mutants examined, strongly supporting the hypothesis that this 2.2 kb transcript is a ced-4 transcript. Total RNA from N2, ced-4(n1162), ced-4(n1416), ced-4 (n1894) and ced-4 (n1920) eggs was probed with 32P-labelled ced-4 cDNA SK2-1. An actin 1 probe (Krause and Hirsh, in: Molecular Biology of the Cytoskeleton, Borisy et al. (eds.), Cold Spring Harbor Laboratory, 1984, pp. 287-292) was used as an internal control for the amount of RNA loaded in each lane. The ratios of the intensity of the ced-4 band to that of actin band in N2, n1162, n1416 and n1894 were 0.5, 0.17, 0 and 0.12, respectively. A Northern blot of poly(A)+ RNA from stage-synchronized animals was probed with pn1416, which hybridizes both to the 2.2 kb ced-4 transcript and to a 0.9 kb transcript. The 0.9 kb transcript seems to be expressed mostly in eggs and adults. The presence of RNA in all lanes was confirmed by loading 1/10 of each sample on another gel and probing a Northern blot from this gel using the C. elegans actin 1 gene (Krause and Hirsh, 1984 supra). That all of these distinct ced-4 mutations cause reduced levels of a ced-4 transcript could reflect either instability of all. three mutant transcripts or a role for ced-4 in regulating its own expression.
Based upon these results, it can be concluded that the 2.2 kb RNA is a ced-4 transcript. It is, not known why the 0.9 kb RNA is also altered in ced-4(n1416) animals. Perhaps transcription of the 0.9 kb RNA is initiated incorrectly as a consequence of the nearby Tc4 element.
ced-4 Expression is Primarily Embryonic
A Northern blot containing RNAs from stage-synchronized animals of different developmental stages probed with pn1416 showed that the 2.2 kb ced-4 transcript was expressed primarily during embryogenesis. This result is consistent with the observation that 113 of the 131 programmed cell deaths in the C. elegans hermaphrodite are embryonic (Sulston and Horvitz, Dev. Biol. 82:110-156 (1977); Sulston et al., Dev. Biol. 100:64-119 (1983)). The 2.2 kb RNA was relatively abundant during embryonic development. The 0.9 kb transcript was expressed mostly in eggs and adults. The presence of RNA in all lanes was confirmed by loading 1/10 of each sample on another gel and probing a Northern blot from this gel with the C. elegans actin 1 gene (Krause and Hirsh, 1984 supra).
The ced-4 Transcript is Present in a ced-3 Mutant
The activities of both ced-3 and ced-4 are required for programmed cell death (Ellis and Horvitz, Cell 44:817-819 (1986)). One possibility is that one of these genes positively regulates the expression of the other. For this reason, a Northern blot of wild-type strain N2 and ced-3(n717) poly(A)+ RNA was probed with pn1416. This experiment showed that the 2.2 kb ced-4 transcript was present at an apparently normal level in this ced-3 mutant. Thus, the activity of the ced-3 gene is unlikely to be necessary for the expression of the ced-4 2.2 kb transcript.
Identification of ced-4 cDNA Clones
To isolate cDNA clones of ced-4, pn1416 was used to probe a C. elegans cDNA phage library made from wild-type strain N2 mixed-stage RNA (Kim and Horvitz, Genes & Dev. 4:357-371 (1990)). Two cDNA clones were isolated. The two cDNA clones (named SK1 and SK2) hybridized to the 2.2 kb ced-4 transcript. Both are about 1.8 kb in size, and both contain one 0.8 kb and one 1.0 kb EcoRI fragment. These EcoRI fragments were subcloned into plasmid vector Bluescribe M13+ (Stratagene). The two subclones derived from SK1 were named SK-1 and SK1-2, and the two subclones derived from SK2 were named SK2-1 and SK2-2. The restriction maps of the SK1- and SK2-derived clones were the same. Sequence analysis of the ends of the four cDNA subclones confirmed the equivalence of the SK1 and SK2 clones, except that SK1-2 contains a poly(A) sequence of more than 50 bp at its 5′ end. This poly(A) sequence is probably a cDNA cloning artifact, since SK1-2 contains the 5′ half of the cDNA (see below).
The ced-4 Sequence
The DNA sequence of the SK2 1.8 kb cDNA clone was. determined. This sequence includes an open reading frame encoding 546 amino acids (FIG. 1; Seq. ID #2), which is consistent with the results of Northern blot analysis using single-stranded RNA probes. An ochre termination codon (TAA) is located in-frame near the 3′ end, indicating that the 3′ end of the 2.2 kb transcript is most likely included in this cDNA. The open reading frame extends to the 5′ end of the 1.8 kb cDNA, suggesting that this cDNA might lack the 5′ end of the ced-4 coding region.
A primer extension experiment was performed to determine the ced-4 transcription initiation site(s) using the primer ATTGGCGATCCTCTCGA (Seq. ID #23) and C10D8-5 as template. A major transcriptional initiation site was identified at 54 bp before (5′ of) the beginning of the ced-4 cDNA SK2 and a minor initiation site at 54 bp after (3′ of) the beginning of this cDNA (FIG. 1). The first AUG codon after the presumptive major start site is located at 9 bp before the beginning of the cDNA (FIG. 1). If this site is used to initiate protein synthesis, the Ced-4 protein would be 549 amino acids in length. The first AUG codon after the presumptive minor start site is located at 130 bp after the beginning of the cDNA. If this site is used, the Ced-4 protein would be 503 amino acids in length. Preliminary results using an anti-Ced-4 antibody raised against a Ced-4 fusion protein showed that endogenous Ced-4 protein is slightly smaller in molecular weight than a Ced-4 fusion protein of 562 amino acids expressed in E. coli. Thus, most Ced-4 protein is probably initiated near the start of the cDNA and is presumably 549 amino acids in length and 62,977 in relative molecular mass. The direction of the open reading frame is consistent with the direction of transcription, as demonstrated by probing Northern blots with single-stranded RNA probes. The presumptive Ced-4 protein is highly hydrophilic, with a pI of 5.12. The longest hydrophobic region is a segment of 12 amino acids from residues 382 to 393.
A Western blot of wild-type strain N2 mixed-stage, ced-4(n1416) mixed-stage, wild-type egg, and bacterially expressed protein (pJ76) was probed using anti-Ced-4 antibody. Ced-4 fusion protein (pJ76) was made by cloning ced-4 cDNA SK2 into the T7 expression vector pET-5a (Rosenberg et al., Gene 56:125-135 (1987)), so that 546 amino acids of Ced-4 sequence were fused to 11 amino acids of T7 gene 10 protein and 5 amino acids of linker sequence. This Ced-4 fusion protein is similar in relative molecular mass to the endogenous Ced-4 protein, which is present in wild-type (N2) but missing in ced-4(n1416) animals. The proteins phosphorylase b, 97×103; bovine serum albumin, 66×103 (Hirayama et al., Biochem. Biophys, Res. Comm. 173:639-646 (1990)); and ovalbumin, 43×103, were used as molecular weight standards.
To confirm the DNA sequence obtained from the ced-4 cDNAs and to study the structure of the ced-4 gene, the sequences of the 4.4 kb cosmid subclone C10DS-5, the 3 kb insert pn1416, and the 2 kb HindIII-BamHI fragment that contains the Tc4 insertion in the ced-4(n1416) mutant were determined. Comparison of the ced-4 genomic and cDNA sequences revealed that the ced-4 gene has seven introns of sizes ranging from 44 bp to 557 bp (FIG. 2). The exon sequences of genomic clone C10D8-5 are identical to the sequences of ced-4 cDNA SK2. Comparison of the Tc4 insertion site in ced-4(n1416) DNA with the ced-4(+) genomic and cDNA sequences indicated that Tc4 inserted into an exon in the ced-4 gene in ced-4(n1416) animals (FIG. 2).
The DNA sequences of eight EMS-induced ced-4 alleles were also determined (Table 2). One of the eight, n1948, is a missense mutation. Of the seven others, four create stop codons and three are predicted to affect splicing of the ced-4 transcript. The positions of these mutations are indicated in FIG. 2. These findings indicate that the phenotypes of these mutants (Ellis and Horvitz, Cell 44:817-829 (1986)) result from a complete loss of ced-4 gene function. These mutations establish the null phenotype of the ced-4 gene, confirming that ced-4 function is not essential for viability.
The Ced-4 Protein Has Two Regions Similar to Known Calcium-Binding Domains
By direct inspection, the sequence of the putative Ced-4 protein was compared with the consensus sequence of the calcium-binding loop of the EF-hand domain (Tufty and Kretsinger, Science 187:161-171 (1975); Kretsinger, Cold spring Harbor Symp. Quant. Biol. 52:499-510 (1987); Szebenyi and Moffat, J. Biol. Chem. 26:8761-8777 (1986)). Two regions of the Ced-4 protein were identified that might bind calcium (FIG. 3).
The EF-hand is a 29 amino acid domain consisting of a helix-loop-helix region, with the loop portion (residues 10-21) coordinating calcium-binding via the side-chain oxygens of serine, threonine, asparagine, aspartic acid, glutamine or glutamic acid. These residues occur at five of the vertices of an octahedron: X (position 10), Y (12), Z (14), −X (18), −Z (21). EF-hand amino acid sequences vary considerably in the residues present in the calcium-binding loop (FIG. 3), and some EF-hand domains have only one helical region (Kretsinger, 1987 supra). The consensus sequence is shown at the top of FIG. 3. Positions Y, Z, and −X can have any of a number of amino acids which have oxygen-containing side chains. Position X is usually aspartic acid, and position −Z is usually glutamic acid.
The sequences of parvalbumins from carp muscle (Seq. ID #3; Nockolds et al., Proc. Natl. Acad. Sci. USA 69:581-584 (1972)), the intestinal calcium-binding protein (ICaBP) (Seq. ID #7-8; Szebenyi et al., Nature 294:327-332 (1981)), troponin C (Seq. ID #9-12; Collins et al., FEBS Lett. 36:268-272 (1973)) and calmodulin (Seq. ID #13; Zimmer et al., J. Biol. Chem. 263:19,370-19,383 (1988); Babu et al., Nature 315:37-40 (1985)) show canonical EF-hands. The hake and ray parvalbumins (Seq. ID #4-5; Capony et al. Eur. J. Biochem. 32:97-108 (1973)); Thatcher and Pechere, Eur. J. Biochem. 75:121-132 (1977)), sarcoplasmic calcium-binding protein (SCBP) from the protochordate Amphioxus (Seq. ID #6; Takagi et al., Biochemistry 25: 3585-3592 (1986)), trypsinogen (Seq. ID #14; Bode and Schwager, J. Mol. Biol. 98:693-717 (1975)), fibrinogen (Seq. ID #15; Doolittle, Ann. Rev. Biochem. 53:195-229 (1984); Dang et al., J. Biol. Chem. 260:9713-9719 (1985)), villin (Seq. ID #16; Hesterberg and Weber, J. Biol. Chem. 258:365-369 (1983)) and galactose-binding protein (GBP) (Seq. ID #17; Vyas et al., Nature 327:635-638 (1987)) show variations from the consensus sequence. GBP does not contain the helices of the EF-hand.
The potential calcium-binding loops of sequence 1 and sequence 2 are located at amino acids 77-88 and amino acids 292-303 of the Ced-4 protein, respectively (FIG. 3). In its putative calcium-binding loop, the first potential EF-hand-like sequence of the Ced-4 protein has four (positions Y, Z, −X, −Z) of the five conserved residues with oxygen-containing side chains (shown in bold), and the fifth position (X) has a tyrosine rather than an aspartic acid; tyrosine contains oxygen in its side chain. The second potential EF-hand-like sequence of the Ced-4 protein has three residues (positions Z, −X, −Z) that match the consensus sequence, and amino acids with oxygen-containing side chains at the other two positions. These observations suggest that these two regions of the Ced-4 protein might bind calcium. Like the Ced-4 protein, a number of known calcium-binding proteins, such a bovine intestinal calcium-binding protein (ICaBP) (Szebenyi and Moffat, 1986 supra), rabbit troponin C (Collins et al., 1973 supra), trypsinogen and villin (Doolittle, 1984 supra; Danget et al., 1985 supra) have only three or four conserved residues at these five positions (FIG. 3). The EF-hand domains in ICaBP and troponin C have been shown by X-ray crystallography to bind calcium.
One major difference between the Ced-4 protein and the calcium-binding loop of the EF-hand consensus sequence is at position 15. Here, the two Ced-4 sequences have a histidine and a glutamic acid, respectively; whereas most ET-hand-containing proteins have a glycine; this glycine has been suggested to be important for the turning of the loop (Kretsinger, 1987 supra). However, a histidine is present at this position in a parvalbumin and an aspartic acid is present in another parvalbumin and also in a sarcoplasmic calcium-binding protein (Kretsinger, 1987 supra) (FIG. 3). Thus, the presence of histidine or glutamic acid at position 15 does not rule out the possibility that these regions bind calcium.
The calcium-binding loop (positions 10-21) of the EF-hand is thought to be preceded (positions 1-9) and followed by alpha-helical domains (positions 22-29) (Kretsinger, 1987 supra). Since position 3 of Ced-4 sequence 1 and positions 26 and 28 of Ced-4 sequence 2 are prolines, these regions might not form alpha-helices. However, the known calcium-binding protein galactose-binding protein (GBP) has a calcium-binding domain similar to that of the EF-hand (FIG. 3) but without the two helices; furthermore, position 29 of GBP is proline (Vyas et al., 1987 supra). Thus, the Ced-4 protein need not contain such alpha-helical calcium-binding domains.
Based upon these considerations, it seems likely that the Ced-4 protein binds calcium or a similar divalent cation.
EXAMPLE 2
CLONING, SEQUENCING, AND CHARACTERIZATION OF THE CED-3 GENE
MATERIALS AND METHODS
General Methods and Strains
The techniques used for the culturing of C. elegans were as described by Brenner (Genetics 77:71-94 (1974)). All strains were grown at 20° C. The wild-type parent strains were C. elegans variety Bristol strain N2, Bergerac strain EM1002 (Emmons et al., Cell 32:55-65 (1983)), C. briggsae and C. vulgaris (obtained from V. Ambros). The genetic markers used are described below. These markers have been described by Brenner (1974 supra), and Hodgkin et al. (In: The Nematode Caenorhabditis elegans, Wood and the Community of C. elegans Researchers (eds.), Cold Spring Harbor Laboratory, 1988, pp 491-584). Genetic nomenclature follows the standard system (Horvitz et al., Mol. Gen. Genet. 175:129-133 (1979)).

    
    
        LG I: ced-1(e1375); unc-54(r323)
        LG VI: unc-31(e928), unc-30(e191), ced-3(n717, n718, n1040, n1129, n1163, n1164, n1165, n1286, n1949, n2426, n2430, n2433), unc-26(e205), dpy-4 (e1166)
        LG V: egl-1(n986); unc-76(e911)
        LG X: dpy-3(e27)

Isolation of Additional Alleles of ced-3

    
    


A non-complementation screen was designed to isolate new alleles of ced-3. Because animals heterozygous for ced-3(n717) in trans to a deficiency are viable (Ellis and Horvitz, Cell 44:817-829 (1986)), animals carrying a complete loss-of-function ced-3, allele generated by mutagenesis were expected to be viable in trans to ced-3(n717), even if the new allele was inviable in homozygotes. Fourteen EMS mutagenized egl-1 males were mated with ced-3 (n717) unc-26(e205); egl-1(n487); dpy-3(e27) hermaphrodites. egl-1 was used as a marker in this screen. Dominant mutations in egl-1 cause the two hermaphrodite specific neurons, the HSNs, to undergo programmed cell death (Trent et al., Genetics 104:619-647 (1983)). The HSNs are required for normal egg-laying, and egl-1(n986) hermaphrodites, which lack HSNs, are egg-laying defective (Trent et al., 1983 supra). The mutant phenotype of egl-1 is suppressed in a ced-3; egl-1 strain because mutations in ced-3 block programmed cell deaths. egl-1 males were mutagenized with EMS and crossed with ced-3(n717), unc-26(e205); egl-1(n487); dpy-3 (e27). Most cross progeny were egg-laying defective because they were heterozygous for ced-3 and homozygous for egl-1. Rare egg-laying competent animals were picked as candidates for carrying new alleles of ced-3. Four such animals were isolated from about 10,000 F1 cross progeny of EMS-mutagenized animals. These new mutations were made homozygous to confirm that they carried recessive mutations of ced-3.
Molecular Biology
Standard techniques of molecular biology were used (Maniatis et al., Molecular Cloning: A Laboratory Manual, Cold Spring Harbor Laboratory, 1983).
Two cosmid libraries were used extensively in this work: a Sau3AI partial digest genomic library of 7000 clones in the vector pHC79 and a Sau3AI partial digest genomic library of 6000 clones in the vector pJB8 (Ish-Horowicz and Burke, Nucleic Acids Res. 9:2989 (1981)).
The “right” end of MMM-C1 was cloned by cutting it with HindIII and self-ligating. The “left” end of MMM-C1 was cloned by cutting it with BglII or SalI and self-ligating.
The “right” end of Jc8 was made by digesting Jc8 with EcoRI and self-ligating. The “left” end of Jc8 was made by digesting Jc8 by SalI and self-ligating.
C. elegans RNA was extracted using guanidine isothiocyanate (Kim and Horvitz, Genes & Dev. 4:357-371 (1990)). Poly(A)+ RNA was selected from total RNA by a poly(dT) column (Maniatis et al., 1983 supra). To prepare stage-synchronized animals, worms were synchronized at different developmental stages (Meyer and Casson, Genetics 106:29-44 (1986)).
For DNA sequencing, serial deletions were made according to a procedure developed by Henikoff (Gene 8:351-359 (1984)). DNA sequences were determined using Sequenase and protocols obtained from US Biochemicals with minor modifications.
The Tc1 DNA probe for Southern blots was pCe2001, which contains a Bergerac Tc1 element (Emmons et al., Cell 32:55-65 (1983)). Enzymes were purchased from New England Biolabs, and radioactive nucleotides were from Amersham.
Primer extension procedures followed the protocol by Robert E. Kingston (In: Current Protocols in Molecular Biology, Ausubel et al. (eds.), Greene Publishing Associates and Wiley-Interscience, New York, p. 4.8.1) with minor modifications.
Polymerase chain reaction (PCR) was carried out using standard protocols supplied by the GeneAmp Kit (Perkin Elmer). The primers used for primer extension and PCR are as follows:

    
    
        Pex2: 5′ TCATCGACTTTTAGATGACTAGAGAACATC 3′ (Seq. ID #24);
        Pex1: 5′ GTTGCACTGCTTTCACGATCTCCCGTCTCT 3′ (Seq. ID #25);
        SL1: 5′ GTTTAATTACCCAAGTTTGAG 3′ (Seq. ID #26);
        SL2: 5′ GGTTTTAACCAGTTACTCAAG 3′ (Seq. ID #27);
        Log5: 5′ CCGGTGACATTGGACACTC 3′ (Seq. ID #28); and
        Oligo10: 5′ ACTATTCAACACTTG 3′ (Seq. ID #29).

Germline Transformation

    
    


The procedure for microinjection basically follows that of A. Fire (EMBO J. 5:2673-2680 (1986)) with modifications: Cosmid DNA was twice purified by CsC1-gradient. Miniprep DNA was used when deleted cosmids were injected. To prepare miniprep DNA, DNA from 1.5 ml overnight bacterial culture in superbroth (12 g Bacto-tryptone, 24 g yeast extract, 8 ml 50% glycerol, 900 ml H2O, autoclaved; after autoclaving, 100 ml 0.17 M KH2PO4 and 0.72 M KH2PO4 were added) was extracted by alkaline lysis method as described in Maniatis et al. (1983 supra). DNA was treated with RNase A (37°, 30 minutes) and then with protease K (55°, 30 minutes), extracted with phenol and then chloroform, precipitated twice (first in 0.3 M sodium acetate and second in 0.1. M potassium acetate, pH 7.2), and resuspended in 5 μl injection buffer as described by A. Fire (1986 supra). The DNA concentration for injection is in the range of 100 ug to 1 mg per ml.
All transformation experiments used ced-1(e1735); unc-31(e928) ced-3(n717) strain. unc-31 was used as a marker for co-transformation (Kim and Horvitz, 1990 supra). ced-1 was present to facilitate scoring of the ced-3 phenotype. The mutations in ced-1 block the engulfment process of cell death, which makes the corpses of the dead cells persist much longer than in wild-type animals (Hedgecock et al., Science 220:1277-1280 (1983)). The ced-3 phenotype was scored as the number of dead cells present in the head of young L1 animals. The cosmid C10D8 or the plasmid subclones of C10D8 were mixed with C14G10 (unc-31(+)-containing) at a ratio of 2:1 or 3:1 to increase the chances that a Unc-31(+) transformant would contain the cosmid or plasmid being tested as well. Usually, 20-30 animals were injected in one experiment. Non-Unc F1 progeny of the injected animal were isolated three to four days later. About 1⁄2 to 1⁄3 of the non-Unc progeny transmitted the non-Unc phenotype to F2 progeny and established a transformant line. The young L1 progeny of such non-Unc transformant were checked for the number of dead cells present in the head using Nomarski optics.
RESULTS
Isolation of Additional ced-3 Alleles
All of the ced-3 alleles that existed previously were isolated in screens designed to detect viable mutants displaying the Ced phenotype (Ellis and Horvitz, Cell 44:817-829 (1986)). Such screens may have systematically missed any class of ced-3 mutations that is inviable as homozygotes. For this reason, a scheme was designed that could isolate recessive lethal alleles of ced-3. Four new alleles of ced-3 (n1163, n1164, n1165, n1286) were isolated in this way. Since new alleles were isolated at a frequency of about 1 in 2500, close to the frequency expected for the generation of null mutations by EMS in an average C. elegans gene (Brenner, Genetics 77:71-94 (1974); Greenwald and Horvitz, Genetics 96:147-160 (1980)), and all four alleles are homozygous viable, it was concluded that the null allele of ced-3 is viable.
Mapping RFLPs near ced-3
Tc1 is a C. elegans transposable element that is thought to be immobile in the common laboratory Bristol strain and in the Bergerac strain (Emmons et al., Cell 32:55-65 (1983)). In the Bristol strain, there are 30 copies of Tc1, while in the Bergerac strain, there are more than 400 copies of Tc1 (Emmons et al., 1983 supra; Finney, Ph.D. thesis, Massachusetts Institute of Technology, Cambridge, Mass., 1987). Because the size of the C. elegans genome is small (haploid genome size 8×107 bp) (Sulston and Brenner, Genetics 77:95-104 (1976)), a polymorphism due to Tc1 between the Bristol and Bergerac strains would be expected to occur about once every 200 kb. Restriction fragment length polymorphisms (RFLPs) can be used as genetic markers and mapped in a manner identical to conventional mutant phenotypes. A general scheme has been designed to map Tc1 elements that are dimorphic between the Bristol and Bergerac strains near any gene of interest (Ruvkun et al., Genetics, 121:501-516 (1989)). Once tight linkage of a particular Tc1 to a gene of interest has been established, that Tc1 can be cloned and used to initiate chromosome walking.
A 5.1 kb Bristol-specific Tc1 EcoRI fragment was tentatively identified as containing the Tc1 closest to ced-3. This Tc1 fragment was cloned using cosmids from a set of Tc1-containing C. elegans Bristol genomic DNA fragments. DNA was prepared from 46 such TC1-containing cosmids, and this DNA was screened using Southern blots to identify the cosmids that contain a 5.1 kb EcoRI Tc1-containing fragment. Two such cosmids were identified: MMM-C1 and MMM-C9. The 5.1 kb EcoRI fragment was subcloned from MMM-C1 into pUC13 (Promega). Since both ends of Tc1 contain an EcoRV site (Rosenzweig et al., Nucleic Acids Res. 11:4201-4209 (1983)), EcoRV was used to remove Tc1 from the 5.1 kb EcoRI fragment, generating a plasmid that contains only the unique flanking region of this Tc1-containing fragment. This plasmid was then used to map the specific Tc1 without the interference of other Tc1 elements.
unc-30(e191) ced-3(n717) dpy-4(e1166)/+++ males were crossed with Bergerac (EM1002) hermaphrodites, and Unc non-Dpy or Dpy non-Unc recombinants were picked from among the F2 progeny. The recombinants were allowed to self-fertilize, and strains that were homozygous for either unc-30(e191) dpy-4(Bergerac) or unc-30(Bergerac) dpy-4(e1166) were isolated. After identifying the ced genotypes of these recombinant strains, DNA was prepared from these strains. A Southern blot of DNA from these recombinants was probed with the flanking sequence of the 5.1 kb EcoRI Tc1 fragment. This probe detects a 5.1 kb fragment in Bristol N2 and a 3.4 kb fragment in Bergerac. Five out of five unc-30 ced-3 dpy(+Berg) recombinants, and one of one unc-30(+Berg) ced-3 dpy-4 recombinants showed the Bristol pattern. Nine of ten unc-30(+Berg) dpy-4 recombinants showed the Bergerac pattern. Only one recombinant of unc-30(+Berg) dpy-4 resulted from a cross-over between ced-3 and the 5.1 kb Tc1 element. The genetic distance between ced-3 and dpy-4 is 2 map units (mu). Thus, this Tc1 element is located 0.1 mu on the right side of ced-3.
Cosmids MMM-C1 and MMM-C9 were used to test whether any previously mapped genomic DNA cosmids overlapped with these two cosmids. A contig of overlapping cosmids was identified that extended the cloned region near ced-3 in one direction.
To orient MMM-C1 with respect to this contig, both ends of MMM-C1 were subcloned and these subclones were used to probe the nearest neighboring cosmid C48D1. The “right” end of MMM-C1 does not hybridize to C48D1, while the “left” end does. Therefore, the “right” end of MM-C1 extends further away from the contig. To extend this contig, the “right” end of MMM-C1 was used to probe the filters of two cosmid libraries (Coulson et al. , Proc. Natl. Acad. Sci. USA 83:7821-7825 (1986)). One clone, Jc8, was found to extend MMM-C1 in the opposite direction of the contig.
RFLPs between the Bergerac and Bristol strains were used to orient the contig with respect to the genetic map. Bristol (N2) and Bergerac (EM1002) DNA was digested with various restriction enzymes and probed with different cosmids to look for RFLPs. Once such an RFLP was found, DNA from recombinants of the Bristol and Bergerac strains between ced-3 and unc-26, and between unc-30 and ced-3 was used to determine the position of the RFLP with respect to ced-3.
The “right” end of Jc8, which represents one end of the contig, detects an RFLP (nP33) when N2 and EM1002 DNA was digested with HindIII. A Southern blot. of DNA from recombinants between three ced-3(+Berg) unc-26 was probed with the “right” end of Jc8. Three of three +Berg unc-26 recombinants showed the Bristol pattern, while two of two ced-3 unc-26(+Berg) recombinants showed the Bergerac pattern. Thus, nP33 mapped very close or to the right side of unc-26.
The “left” end of Jc8 also detects a HindIII RFLP (nP34). The same Southern blot was reprobed with the Jc8 “left” end. Two of the two ced-3 unc-26(+Berg) recombinants and two of the three ced-3(+Berg) unc-26 recombinants showed the Bergerac pattern. One of the three ced-3(+Berg) unc-26 recombinants showed the Bristol pattern. The genetic distance between ced-3 and unc-26 is 0.2 mu. Thus, nP34 was mapped between ced-3 and unc-26, about 0.1 mu on the right side of ced-3.
The flanking sequence of the 5.1 kb EcoRI Tc1 fragment (named nP35) was used to probe the same set of recombinants. Two of three ced-3(+Berg) unc-26 recombinants and two of two ced-3 unc-26(+Berg) recombinants showed the Bristol pattern. Thus, nP35 was also found to be located between ced-3 and unc-26, about 0.1 mu on the right side of ced-3.
A similar analysis using cosmid T10H5 which contains the HindIII RFLP (nP36), and cosmid B0564, which contains a HindIII RFLP (nP37), showed that nP36 and nP37 mapped very close or to the right of unc-30.
These experiments localized the ced-3 gene to an interval of three cosmids. The positions of the RFLPs, and of ced-3, unc-30 and unc-26 on chromosome IV, and their relationships to the cosmids are shown in FIG. 9. It was has been further demonstrated by microinjection that cosmids C37G8 and C33F2 carry the unc-30 gene (John Sulston, personnel communication). Thus, the region containing the ced-3 gene was limited to an interval of two cosmids. These results are summarized in FIG. 9.
Complementation of ced-3 by Germline Transformation
Cosmids that were candidates for containing the ced-3 gene were microinjected into a ced-3 mutant to see if they rescue the mutant phenotype. The procedure for microinjection was that of A. Fire (EMBO J. 5:2673-2680 (1986)) with modifications. unc-31, a mutant defective in locomotion, was used as a marker for cotransformation (Kim and Horvitz, Genes & Dev. 4:357-371 (1990)), because the phenotype of ced-3 can be examined only by using Nomarski optics. Cosmid C14G10 (containing unc-31(+)) and a candidate cosmid were coinjected into ced-l e1375); unc-31 (e928) ced-3 (n717) hermaphrodites, and F1 non-Unc transformants were isolated to see if the non-Unc phenotype could be transmitted and established as a line of transformants. Young L1 progeny of such transformants were examined for the presence of cell deaths using Nomarski optics to see whether the ced-3 phenotype was suppressed. Cosmid C14G10 containing unc-31 alone does not rescue ced-3 activity when injected into a ced-3 mutant. Table 4 summarizes the results of these transformation experiments.
As shown in Table 4, of the three cosmids injected (C43C9, W07H6 and C48D1), only C48D1 rescued the ced-3 phenotype (2/2 non-Unc transformants rescued the ced-3 phenotype). One of the transformants, nEX2, appears to be rescued by an extra-chromosomal array of injected cosmids (Way and Chalfie, Cell 54:5-16 (1988)), which is maintained as an unstable duplication, since only 50% of the progeny of a non-Unc Ced(+) animal are non-Unc Ced(+). Since the non-Unc Ced(+) phenotype of the other transformant (nIS1) is transmitted to all of its progeny, it is presumably an integrated transformant. L1 ced-1 animals contain an average of 23 cell corpses in the head (Table 5). L1 ced-1; ced-3 animals contain an average of 0.3 cell corpses in the head. ced-1; unc-31 ced-3; nIS1 and ced-1; unc-31 ced-3; nEX2 animals contain an average of 16.4 and 14.5 cell corpses in the head, respectively. From these results, it was concluded that C48D1 contains the ced-3 gene.
In order to locate ced-3 more precisely within the cosmid C48D1, this cosmid was subcloned and the subclones were tested for the ability to rescue ced-3 mutants (Table 5). C48D1 DNA was digested with restriction enzymes that cut rarely within the cosmid and the remaining cosmid was self-ligated to generate a subclone. Such subclones were then injected into a ced-3 mutant to look for complementation; young L1 non-Unc progeny of the transformants were examined using Nomarski optics for the presence of cell death in the head. When C48D1 was digested with BamHI and self-ligated, the remaining 14 kb subclone (named C48D1-28) was found to rescue the ced-3 phenotype when injected into a ced-3 mutant (FIG. 10 and Table 5). C48D1-28 was then partially digested with BglII and self-ligated. Clones of various lengths were isolated and tested for their ability to rescue ced-3.
One clone, C48D1-43, which did not contain a 1.7 kb BglII fragment of C48D1-28, was able to rescue ced-3 (FIG. 10 and Table 5). C48D1-43 was further subcloned by digesting with BamHI and ApaI to isolate a. 10 kb BamHI-ApaI fragment. This fragment was subcloned into pBSKII+ to generate pJ40. pJ40 can restore ced-3+ phenotype when microinjected into a ced-3 mutant. pJ40 was subcloned by deleting a 2 kb BglII-ApaI fragment to generate pJ107. pJ107 was also able to rescue the ced-3 phenotype when microinjected into a ced-3 mutant. Deletion of 0.5 kb on the left side of pJ107 could be made by ExoIII digestion (as in pJ107del28 and pJ107del34) without affecting ced-3 activity; in fact, one transgenic line, nEX17, restores full ced-3 activity. However, the ced-3 rescuing ability was significantly reduced when 1 kb was deleted on the left side of pJ107 (as in pJ107del12 and pJ107del27), and the ability was completely eliminated when a 1.8 kb SalI-BglII fragment was deleted on the right side of pJ107 (as in pJ55 and pJ56), suggesting that this SalI site is likely to be in the ced-3 coding region. From these experiments, ced-3 was localized to a DNA fragment of 7.5 kb. These results are summarized in FIG. 10 and Table 5.
ced-3 Transcript
pJ107 was used to probe a Northern blot of N2 RNA and detected a band of 2.8 kb. Although this transcript is present in 12 ced-3 mutant animals, subsequent analysis showed that all 12 ced-3 mutant alleles contain mutations in the genomic DNA that codes for this mRNA (see below), thus establishing this RNA as a ced-3 transcript.
The developmental expression pattern of ced-3 was determined by hybridizing a Northern blot of RNA from animals of different stages (eggs, L1 through L4 larvae and young adult) with the ced-3 cDNA subclone pJ118. Such analysis revealed that the ced-3 transcript is most abundant during embryonic development, which is the period when most programmed cell deaths occur, but it was also detected during the L1 through L4 larval stages and is present in relatively high levels in young adults. This result suggests that ced-3 is not only expressed in cells undergoing programmed cell death.
Since ced-3 and ced-4 are both required for programmed cell death in C. elegans, one of the genes might-act as a regulator of transcription of the other gene. To examine if ced-4 regulates the transcription of ced-3, RNA was prepared from eggs of ced-4 mutants (n1162, n1416, n1894, and n1920), and a Northern blot was probed with the ced-3 cDNA subclone pJ118. The presence of RNA in each lane was confirmed with an actin I probe. Such an experiment showed that the level of ced-3 transcript is normal in ced-4 mutants. This indicates that ced-4 is unlikely to be a transcriptional regulator of ced-3.
Isolation of a ced-3 cDNA
To isolate cDNA of ced-3, pJ40 was used as a probe to screen a cDNA library of N2 (Kim and Horvitz, Genes & Dev. 4:357-371 (1990)). Seven cDNA clones were isolated. These cDNAs can be divided into two groups: one is 3.5 kb and the other 2.5 kb. One cDNA from each group was subcloned and analyzed further. pJ85 contains the 3.5 kb cDNA. Experiments showed that pJ85 contains a ced-3 cDNA fused to an unrelated cDNA; on Northern blots of N2 RNA, the pJ85 insert hybridizes to two RNA transcripts, and on Southern blots of N2 DNA, pJB5 hybridizes to more than one band than pJ40 (ced-3 genomic DNA) does. pJ87 contains the 2.5 kb cDNA. On Northern blots, pJ87 hybridizes to a 2.8 kb RNA and on Southern blots, it hybridizes only to bands to which pJ40 hybridizes. Thus, pJ87 contains only ced-3 cDNA.
To show that pJ87 does contain the ced-3 cDNA, a frameshift mutation was made in the Sa1I site of pJ40 corresponding to the SalI site in the pJ87 cDNA. Constructs containing the frameshift mutation failed to rescue the ced-3 phenotype when microinjected into ced-3 mutant animals, suggesting that ced-3 activity has been eliminated.
ced-3 Sequence
The DNA sequence of pJ87 was determined (see FIG. 4; Seq. ID #18). pJ87 contains an insert of 2.5 kb which has an open reading frame of 503 amino acids (FIG. 4; Seq. ID #19). The 5′ end of the cDNA. contains 25 bp of poly-A/T sequence, which is probably an artifact of cloning and is not present in the genomic sequence. The cDNA ends with a poly-A sequence, suggesting that it contains the complete 3′ end of the transcript. 1 kb of pJ87 insert is untranslated 3′ region and not all of it is essential for ced-3 expression, since genomic constructs with deletions of 380 bp of the 3′ end can still rescue ced-3 mutants (pJ107 and its derivatives, see FIG. 10).
To confirm the DNA sequence obtained from the ced-3 cDNA and to study the structure of the ced-3 gene, the genomic sequence of the ced-3 gene in the plasmid pJ107 was determined (FIG. 4; Seq. ID #18). Comparison of the ced-3 genomic and cDNA sequences revealed that the ced-3 gene has seven introns that range in size from 54 bp to 1195 bp (FIG. 5A). The four largest introns, as well as sequences 5′ of the start codon, were found to contain repetitive elements. Five types of repetitive elements were found, some of which have been previously characterized in non-coding regions of other C. elegans genes such as fem-1 (Spence et al., Cell 60:981-990 (1990)), lin-12 (J. Yochem, personal communication), and myoD (Krause et al., Cell 63:907-919(1990)) (FIG. 4). Of these, repeat 1 was also found in fem-1 and myoD, repeat 3 in lin-12 and fem-1, repeat 4 in lin-12, and repeats 2 and 5 were novel repetitive elements.
A combination of primer extension and PCR amplification was used to determine the location and nature of the 5′ end of the ced-3 transcript. Two primers (Pex1 and Pex2) were used for the primer extension reaction. The Pex1 reaction yielded two major bands, whereas the Pex2 reaction gave one band. The Pex2 band corresponded in size to the smaller band from the Pex1 reaction, and agreed in length with a possible transcript that is trans-spliced to a C. elegans splice leader (Bektesh, Genes & Dev., 2:1277-1283 (1988)) at a consensus splice acceptor at position 2166 of the genomic sequence (FIG. 4). The nature of the larger Pex1 band is unclear.
To confirm the existence of this trans-spliced message in wild-type worms, total C. elegans RNA was PCR amplified using the SL1-Log5 and SL2-Log5 primer pairs, followed by a reamplification using the SL1-oligo10 and SL2-Oligo10 primer pairs. The SL1 reaction yielded a fragment of the predicted length. The identity of this fragment was confirmed by sequencing. Thus, at least some, if not most, of the ced-3 transcript is trans-spliced to SL1. Based on this result, the start codon of the ced-3 message was assigned to the methionine encoded at position 2232 of the genomic sequence (FIG. 4).
The DNA sequences of 12 EMS-induced ced-3 alleles were also determined (FIG. 4 and Table 3). Nine of the 12 are missense mutations. Two of the 12 are nonsense mutations, which might prematurely terminate the translation of ced-3. These nonsense ced-3 mutants confirmed that the ced-3 gene is not essential for viability. One of the 12 mutations is an alteration of a conserved splicing acceptor G, and another has a change of a 70% conserved C at the splice site, which could also generate a stop codon even if the splicing is correct. Interestingly, these EMS-induced mutations are in either the N-terminal quarter or C-terminal-half of the protein. In fact, 9 of the 12 mutations occur within the region of ced-3 that encodes the last 100 amino acids of the protein. Mutations are notably absent from the middle part of the ced-3 gene (FIG. 5).
Ced-3 Protein Contains A Region Rich in Serines
The Ced-3 protein is very hydrophilic and no significantly hydrophobic region can be found that might be a trans-membrane domain (FIG. 6). The Ced-3 protein is rich in serine. From amino acid 78 to amino acid 205 of the Ced-3 protein, 34 out of 127 amino acids are serine. Serine is often the target of serine/threonine protein kinases (Edelman, Ann. Rev. Biochem. 56:567-613 (1987)). For example, protein kinase C can phosphorylate serines when they are flanked on their amino and carboxyl sides by basic residues (Edelman, 1987 supra). Four of the serines in the Ced-3 protein are flanked by arginines (FIG. 4). The same serine residues might also be the target of related Ser/Thr kinases.
To identify the functionally important regions of the Ced-3 protein, genomic DNAs containing the ced-3 genes from two related nematode species, C. briggsae and C. vulgaris were cloned and sequenced (FIG. 7; Seq. ID #20 and 21). Sequence comparison of the three ced-3 genes showed that the non-serine-rich region of the proteins is highly conserved. In C. briggsae and C. vulgaris, many amino acids in the serine-rich region are dissimilar compared to the C. elegans Ced-3 protein (FIG. 7). It seems that what is important in the serine-rich region is the overall serine-rich feature rather than the exact amino acid sequence.
This hypothesis is also supported by analysis of ced-3 mutations in C. elegans: none of the 12 EMS-induced mutations is in the serine-rich region, suggesting that mutations in this region might not affect the function of the Ced-3 protein and thus, could not be isolated in the screen for ced-3 mutants.







TABLE 1







Rescue of the Ced-4


Phenotype by Germline Transformation















No.




DNA
Avg. No. Cell
Animals



Genotype
Injected
Corpses (L1 Head)
Scored
















ced-1; ced-4;
C10D8;
9.4
10



unc-31; nEx1
C14G10



ced-1; ced-4;
C10D8-5
11.5
10



unc-31; nEx7
C14G10



ced-1; ced-4
C10D8-5
11.5
10



unc-31; nEx8
C14G10



ced-1
None
23
20



ced-1; ced-4
None
0.6
20

















TABLE 2







Sites of Mutations in the ced-4 Gene











Allele
Mutation
Nucleotide
Codon
Consequence





n1162
C to T
1131
40
Q to ochre (TAA)


n2274
C to T
1428
139
R to opal (TGA)


n1920 &
G to A
1744
first base of 5′
Altered splicing


n2247


splice donor of





intron 3


n2273
G to A
1929
first base of 3′
Altered splicing





splice acceptor of





intron 3


n1948
T to A
2117
258
I to N


n1947
C to T
2128
262
Q to amber


n1894
G to A
3131
401
W to opal (TGA)





Nucleotide and codon positions correspond to the numbering in FIG. 1. 













TABLE 3







Sites of Mutations in the ced-3 Gene











Allele
Mutation
Nucleotide
Codon
Consequence














n1040
C to T
2310
27
L to F


n718 
G to A
2487
65
G to R


n2433
G to A
5757
360
G to S


n1164
C to T
5940
403
Q to termination


n717 
G to A
6297
—
Splice acceptor






loss


n1949
C to T
6322
412
Q to termination


n1286
G to A
6342
428
W to termination


n1129
C to T
6434
449
A to V


n1165
C to T
6434
449
A to V


n2430
C to T
6485
466
A to V


n2426
G to A
6535
483
E to K


n1163
C to T
7020
486
S to F





Nucleotide and codon positions correspond to the numbering in FIG. 4. 













TABLE 4







Summary of Transformation Experiments


Using Cosmids in the ced-3 Region










Cosmid
No. of non-Unc
Ced-3



injected
transformants
phenotype
Strain name





C43C9; C14G10
1
−
MT4302


W07H6; C14G10
3
−
MT4299




−
MT4300




−
MT4301


C48D1; C14G10
2
+
MT4298




+
MT4303





Animals injected were of genotype: ced-1(e1735); unc-31(e929) ced-3(n717). 













TABLE 5







The expression of ced-3(+) transformants














Average No.
No.





cell deaths
Animals



Genotype
DNA injected
in L1 head
scored
















ced-1
—
23
20



ced-1; ced-3
—
0.3
10



ced-1; nIS1
C48D1;
16.4
20



unc-31 ced-3
C14G10



ced-1; unc-31

14.5
20



ced-3; nIS1/+



ced-1; unc-31
C48D1;
13.2
10/14



ced-3; nEX2
C14G10
0
 4/14



ced-1; unc-31
C48D1-28;
12
 9/10



ced-3; nEX10
C14G10
0
1 of 10



ced-1; unc-31
C48D1-28;
12
10



ced-3; nEX9
C14G10



ced-1; unc-31
C48D1-43
16.7
10/13



ced-3; nEX11
C14G10
Abnormal cell
 3/13





deaths



ced-1; unc-31
pJ40; C14G10
13.75
4/4



ced-3; nEX13



ced-1; unc-31
pJ107de128,
23
12/14



ced-3; nEX17
pJl07de134
0
 2/14




C14G10



ced-1; unc-31
pJ107de128,
12.8
 9/10



ced-3; nEX18
pJ107de1134
0
 1/10




C14G10



ced-1; unc-31
pJ107de128,
10.6
5/6



ced-3; nEX19
pJ107de134
0
1/6




G14G10



ced-1; unc-31
pJ107de112,
7.8
12/12



ced-3; nEX16
pJ107de127




C14G10







Alleles of the genes used are ced-1(e1735), unc-31(e928), and ced-3(n717). 






Equivalents

Those skilled in the art will recognize, or be able to ascertain using no more than routine experimentation, many equivalents to the specific embodiments of the invention described herein. Such. equivalents are intended to be encompassed by the following claims. For example, functional equivalents of DNAs and RNAs may be nucleic acid sequences which, through the degeneracy of the genetic code, encode the same proteins as those specifically claimed. Functional equivalents of proteins may be substituted or modified amino acid sequences, wherein the substitution or modification does not change the activity or function of the protein. A “silent” amino acid substitution, such that a chemically similar amino acid (e.g., an acidic amino acid with another acidic amino acid) is substituted, is an example of how a functional equivalent of a protein can be produced. Functional equivalents of nucleic acids or proteins can also be produced by deletion of nonessential sequences.

## Claims

1. An isolated protein comprising the amino acid sequence of SEQ ID NO.:19.

2. The isolated polypeptide of claim 1, wherein said polypeptide consists of the amino acid sequence of SEQ. ID NO.:19.