The Caenorhabditis elegans Dosage Compensation Machinery Is Recruited to X Chromosome DNA Attached to an Autosome
Jason D. Lieb, Carlos Ortiz de Solorzano, Enrique Garcia Rodriguez, Arthur Jones, Michael Angelo, Stephen Lockett, Barbara J. Meyer

Abstract

The dosage compensation machinery of Caenorhabditis elegans is targeted specifically to the X chromosomes of hermaphrodites (XX) to reduce gene expression by half. Many of the trans-acting factors that direct the dosage compensation machinery to X have been identified, but none of the proposed cis-acting X chromosome-recognition elements needed to recruit dosage compensation components have been found. To study X chromosome recognition, we explored whether portions of an X chromosome attached to an autosome are competent to bind the C. elegans dosage compensation complex (DCC). To do so, we devised a three-dimensional in situ approach that allowed us to compare the volume, position, and number of chromosomal and subchromosomal bodies bound by the dosage compensation machinery in wild-type XX nuclei and XX nuclei carrying an X duplication. The dosage compensation complex was found to associate with a duplication of the right 30% of X, but the complex did not spread onto adjacent autosomal sequences. This result indicates that all the information required to specify X chromosome identity resides on the duplication and that the dosage compensation machinery can localize to a site distinct from the full-length hermaphrodite X chromosome. In contrast, smaller duplications of other regions of X appeared to not support localization of the DCC. In a separate effort to identify cis-acting X recognition elements, we used a computational approach to analyze genomic DNA sequences for the presence of short motifs that were abundant and overrepresented on X relative to autosomes. Fourteen families of X-enriched motifs were discovered and mapped onto the X chromosome.

DOSAGE compensation is an essential, chromosome-wide regulatory process that equalizes expression of most X-linked genes between males (usually XO or XY) and females (usually XX), despite their two-fold difference in X chromosome dose. Flies, worms, and mammals utilize diverse mechanisms of dosage compensation, but all involve global changes in X chromosome structure that ultimately serve to adjust the level of X-linked transcripts in only one sex (Cline and Meyer 1996; Meller 2000; Meyer 2000). These X chromosome changes are mediated by dosage compensation machinery that must recognize and associate specifically with the X chromosome(s) of only the dosage-compensating sex. Although the identity and properties of proteins and noncoding RNAs that execute dosage compensation are known in detail, much less is known about the cis-acting factors that must reside on the X chromosome to recruit the dosage compensation machinery. Important advances in understanding the problem of X chromosome recognition have come from analysis of dosage compensation in mammals and Drosophila melanogaster.

Female placental mammals (XX) inactivate one of their two X chromosomes to achieve levels of X chromosome expression equal to those of the XY male (Lee and Jaenisch 1997). The inactivated mammalian X chromosome is hypoacetylated, hypermethylated, and hypercondensed to form a structure called the Barr body (Lyon 1961; Mohandaset al. 1981; Jeppesen and Turner 1993). X inactivation is initiated at a small cis-acting locus on the X chromosome, the X inactivation center (Xic; Lee et al. 1996, 1999; Herzinget al. 1997), which has been localized to an 80-kb fragment that can confer inactivation properties onto autosomes (Leeet al. 1999). Encoded within the Xic is a noncoding RNA called Xist, which helps to choose the specific X chromosome(s) to be inactivated (Marahrenset al. 1998) and then spreads in cis along the future inactive X (Clemsonet al. 1996; Pennyet al. 1996). Although Xist is not required for the maintenance of the inactive state (Csankovszkiet al. 1999), it may function to recruit specialized repressive chromatin components to X at the onset of inactivation (Brown and Willard 1994; Lee and Jaenisch 1997). Regulation of Xist and hence X inactivation is achieved in part by a noncoding 40-kb transcript called Tsix that is antisense to and spans the Xist gene. A female X chromosome that cannot transcribe Tsix is destined to be inactivated, suggesting that Tsix is involved in X chromosome choice and negatively regulates Xist (Lee and Lu 1999). Together these studies indicate that the Xist locus serves as the primary cis-acting element in X chromosome recognition and that the dosage compensation machinery associates with X by a nucleation and spreading mechanism. Furthermore, no broadly distributed X-specific sequences are required for Xist binding or propagation.

In contrast to mammals, Drosophila males (XY) compensate for their lower X chromosome dose by hypertranscribing their single X. Dosage compensation is implemented by the male-specific lethal genes msl1, msl2, msl3, mle, and mof whose products form a complex that associates specifically with hundreds of sites along the male X chromosome (Kurodaet al. 1991; Palmeret al. 1993; Gorman et al. 1993, 1995; Bashaw and Baker 1995; Kelleyet al. 1995; Zhouet al. 1995). In flies mutant for an msl gene, partial MSL complexes localize to a subset (30-40) of sites along the X (Palmeret al. 1994; Gormanet al. 1995; Lymanet al. 1997; Guet al. 1998). In a surprising parallel to mammalian dosage compensation, an RNA component was discovered in the Drosophila dosage compensation machinery. Two untranslated RNAs, roX1 and roX2, colocalize to the male X chromosome in an MSL complex-dependent manner (Amrein and Axel 1997; Melleret al. 1997). The roX1 and roX2 loci themselves correspond to two of the sites that retain MSL binding in msl mutants (Kelleyet al. 1999). Unlike individual X-derived genes that fail to retain MSL binding when moved to autosomes (Bone and Kuroda 1996; Bhadraet al. 1999), the roX1 gene can recruit MSL proteins to autosomes, and the proteins can then spread onto flanking autosomal genes (Kelleyet al. 1999). These results suggest that roX genes are X chromatin entry sites for the dosage compensation machinery (Kelleyet al. 1999). Thus, Drosophila appears to use a discrete set of entry sites positioned along the X chromosome to recruit the dosage compensation machinery and permit spreading to adjacent genes. The properties of the entry sites that confer the MSL recruitment activity are as yet not understood.

In the nematode Caenorhabditis elegans, hermaphrodites (XX) reduce the level of transcripts from each of their two X chromosomes by half to equal the expression from the single male X (Meyer and Casson 1986; Plenefischet al. 1989; Chuanget al. 1994). Failure to activate dosage compensation in hermaphrodites results in overexpression of X-linked genes and lethality (Nusbaum and Meyer 1989; Plenefischet al. 1989; Meyer 1997). C. elegans dosage compensation is implemented by a protein complex that localizes specifically to both X chromosomes of hermaphrodites at about the 40-cell stage of embryogenesis (Figure 1; Chuang et al. 1994, 1996; Lieb et al. 1996, 1998). This biochemically and genetically defined dosage compensation complex (DCC) includes proteins specific to dosage compensation (DPY-27) and proteins that also function in chromosome segregation during mitosis (MIX-1) or meiosis (DPY-26 and DPY-28; Chuang et al. 1994, 1996; Lieb et al. 1996, 1998). DPY-27 and MIX-1 are members of the highly conserved SMC family of proteins, which includes proteins that participate in diverse chromosome behaviors including sister chromatid cohesion, mitotic chromosome condensation, and mitotic recombination repair (Chuanget al. 1994; Koshland and Strunnikov 1996; Liebet al. 1998). DPY-26 has two small motifs in common with two mitotic proteins: XCAP-H, a component of the Xenopus laevis 13S condensin complex (Hirano et al. 1997), and Barren, a Drosophila protein essential for mitotic chromosome segregation in vivo (Bhatet al. 1996). Although DPY-26 is required for the faithful segregation of chromosomes during meiosis (Hodgkin 1983), it has diverged significantly from both homologs and does not appear to function in mitosis (Liebet al. 1996). The X localization of DPY-26, DPY-27, and MIX-1, and their similarity to proteins involved in chromosome dynamics, led to the view that the dosage compensation complex regulates gene expression by altering X chromosome structure.

Individually, DPY-26, DPY-27, DPY-28, and MIX-1 cannot associate with X, nor can a complex containing all four proteins (Hsuet al. 1995; Chuanget al. 1996; Lieb et al. 1996, 1998). Instead, the hermaphrodite-specific proteins SDC-2 and SDC-3 are required for assembling the complex on X (Chuanget al. 1996; Davis and Meyer 1997). SDC-2 activates the dosage compensation process and confers hermaphrodite specificity: its product is present exclusively in XX animals and its ectopic expression in males causes inappropriate dosage compensation and death, unlike any other dosage compensation protein (Nusbaum and Meyer 1989; Daweset al. 1999). SDC-2 may also direct X recognition, since it can localize to the X in the absence of the other known DCC components or dosage compensation genes. Several lines of evidence indicate that SDC-2 collaborates with SDC-3 to target the dosage compensation machinery to X. SDC-3 also associates with X, it contains a pair of TFIIIA-type zinc-finger motifs that are essential for assembly of the DCC on X, and it acts synergistically with SDC-2 to kill males when overexpressed (DeLonget al. 1993; Klein and Meyer 1993; Davis and Meyer 1997; Daweset al. 1999).

A reasonable hypothesis for X recognition is that cis-acting DNA elements on the C. elegans X chromosome allow trans-acting factors like the SDC proteins to associate with X and thereby recruit the dosage compensation machinery. Such elements have not yet been identified. X recognition has been particularly difficult to approach in C. elegans because of a lack of candidate X recognition elements, the inability to make directed chromosomal insertions or deletions, and the extremely small size of somatic chromosomes. In this study, two general strategies were pursued in an attempt to overcome these obstacles and to identify and isolate cis-acting X recognition elements. The first was to determine whether portions of the X chromosome attached to an autosome are competent to bind the dosage compensation complex, and if so whether this binding spreads into the autosomal region. This was accomplished with a novel three-dimensional in situ approach that allowed us to compare the volume, position, and number of DCC foci between wild-type nuclei and nuclei homozygous for autosome-attached duplications of different portions of X. The second strategy utilized a computational approach to identify X chromosome-enriched sequence motifs.

Figure 1.

—A model for assembly of the dosage compensation complex on hermaphrodite X chromosomes in C. elegans. (A) In XX hermaphrodites, SDC-2 acts in conjunction with SDC-3 to activate dosage compensation by localizing a protein complex composed of DPY-26, DPY-27, DPY-28, and MIX-1 to both hermaphrodite X chromosomes. The end result is an approximately twofold reduction in X-linked gene expression from each X chromosome. (B) In XO males, the DCC is prevented from associating with X because the male-specific xol-1 gene represses sdc gene activity. X-linked genes are fully expressed because the dosage compensation proteins are prevented from localizing to the single X.

MATERIALS AND METHODS

Strains: Animals were maintained on NG agar plates with Escherichia coli OP50 as a food source (Brenner 1974). The following strains were used in this study:

TY0125
wild type (N2)
SP0117
mnDp10(X;I); unc-3(e151) X
TY2025
yDp14(X;I); unc-2(e55) X
SP0076
mnDp27(X;II); unc-3(e151) X
TY0689
stDp2(X;II); dpy-6(e14) X.

Antibody staining: For each experiment, wild-type and duplication-bearing embryos were prepared in parallel using identical reagents, and the samples were subjected to confocal microscopy on the same day. Gravid adult worms (10-30) were transferred to a positively charged glass slide (Permafrost Plus; Fisher Scientific, Pittsburgh, PA) in 6 μl of M9 buffer. An incision was made at the vulva to release the embryos. An 18 × 18 mm coverslip was placed on top of the sample, and the slide was placed directly on a block of dry ice for at least 10 min. The coverslip was then removed from the slide with a quick downward stroke of a single-edged razor. The slide was immediately placed in 95% ethanol for 1 min and then incubated in PBS for 5 min. Most of the PBS was wicked away, and 50 μl of fixative [4% paraformaldehyde, 18% methanol, 3 mm EGTA, 64 mm KCl, 16 mm NaCl, 0.4 mm spermidine-HCl, 0.16 mm spermine, 0.4% β-mercaptoethanol, 12 mm PIPES (pH 7.4)] was placed directly on the sample and covered with a 30 × 30 mm piece of parafilm. The slides were then placed on ice for 20-30 min. The fixative was removed from the samples by placing the slide into a vessel containing PBS (15 min) and washed 15 min in PBSTB (1 × PBS, 0.1% BSA, 0.5% Tween 20, 0.05% azide, 1 mm EDTA), and 15 min in PBSTA (1 × PBS, 1% BSA, 0.5% Tween 20, 0.05% sodium azide, 1 mm EDTA). A 30-μl dilution of the primary antibody in PBSTA (1:100) was then placed on the sample, which was covered with a 30 × 30 mm piece of parafilm. The slide was placed in a humidified chamber for 4 hr at room temperature. The slides were washed as before and the secondary antibody was applied in the same manner as the primary. After washing as before, 200 μg/ml RNase was then placed on samples, which were incubated at 37° for 1 hr. The samples were washed and incubated with 2 μg/ml propidium iodide for 1 hr, washed, and mounted for confocal microscopy. An N-propyl gallate/glycerol mix (2% n-propyl galate, 30 mm Tris-HCl pH 9.5, 70% glycerol) was used as an antifade reagent in the mount.

Detection of extrachromosomal arrays: Wild-type worms were transformed with pRF4, a plasmid encoding rol-6(su1006) (a marker for transgenic worms), pSV2-dhFr8.32, a plasmid containing 32 copies of tandem lacO repeats (Straightet al. 1996; Carmiet al. 1998; Daweset al. 1999), and pPD49-78, which expresses lactose repressor-green fluorescent protein (LACI-GFP) under control of the hsp-16 heat-shock promoter (A. Gonzalez-Serricchio and P. Sternberg, personal communication). Worms were raised at 20°, heat shocked for 30 min at 37° to express LACI-GFP, and allowed to recover for 30 min at 20°. The LACI-GFP binds to the lac operator sequences in the array, allowing the extrachromosomal arrays to be detected by antibodies to GFP. The worms were then prepared for microscopy as described above except their DNA was stained with 50 μg/ml of diamidinophenolindole (DAPI) included in 1,4-diazobicyclo(2,2,2)octane/glycerol mount at neutral pH.

Figure 2.

—Three-dimensional reconstruction of fluorescence in wild-type embryonic nuclei. (A-C) The 3-D reconstruction of anti-DPY-27 staining in a single nucleus. The black plane is a single section of original confocal data, and the blue objects are surface renderings based on the position of the edges of fluorescence in stacks of optical sections. The algorithms used to render and segment the DPY-27-labeled X chromosomes produced a 3-D body that was representative of the original data. All transformations of the raw confocal data (image filters, interpolation, and settings used for rendering) were identical for all samples analyzed in this article. (D-F) Surface rendering of the DNA stain propidium iodide. daVinci, the software used to render the nuclei, allows one to adjust the opacity of the rendered DNA stain, permitting one to visualize the position of staining bodies inside the nuclei. (D) 0% opacity, (E) 25% opacity, (F) 100% opacity. (G-I) Subchromosomal pieces of DNA can be detected and resolved from the X chromosomes. (G) A wild-type embryo harboring an array composed of the lacO, lacI-GFP, and rol-6 plasmids was stained with anti-GFP (FITC, green), anti-DPY-27 (CY5, red), and DAPI (blue). A merged image of a single optical section is shown. (H and I) 3-D reconstructions of extrachromosomal arrays (red), DPY-27-stained X chromosomes (dark blue), and DAPI staining (light blue) from 2 individual nuclei are shown. This embryo had 179 nuclei and 220 arrays. Fourteen (7.8%) nuclei contained 0 arrays, 115 (64.2%) nuclei contained 1 array, 45 (25.1%) nuclei contained 2 arrays, and 5 (2.8%) nuclei contained 3 arrays. (J) The two X chromosomes often appear as one body of staining. These three nuclei are examples in which the two X chromosomes are counted as one staining body. C. elegans embryonic nuclei are generally 1-2 μm in diameter.

Microscopy: For experiments using duplications, microscopy was carried out on a Zeiss 410 confocal microscope (experiments 1 and 2) or a Leica TCS NT confocal (experiments 3 and 4). For array experiments, microscopy was performed on the Leica confocal microscope. All images were acquired with a 63× oil-immersion objective (numerical aperture = 1.32) at a zoom of 3 with a 512 × 512 image size; pinhole = 1. Photomultiplier settings were determined automatically by the computer (Zeiss) or determined manually using the “glow over” look-up table (Leica). For the Leica, photomultiplier tube settings were adjusted to maximize signal intensity but minimize saturated pixels. The gain/offset was not adjusted from the default values (a black background was produced). Individual sections were averaged four times in “frame” mode. The step size in the z direction was 300 nm (Zeiss) or 283 nm (Leica), creating voxels of X = 102 nm, Y = 102 nm, Z = 300 or 283 nm. At an excitation wavelength of 488 nm (for fluorescein isothiocyanate) the microscopes used in this study have a maximum theoretical xy resolution of ∼225 nm, and a maximum theoretical z resolution of ∼280 nm (using an ∼140 nm z-step size). In these experiments, a z-step size of 300 nm was used as a compromise between optimal resolution in z, photo-bleaching effects, and image file size. A 300-nm step size translates into ∼60 raw data slices per embryo and between three and four raw data slices per nucleus.

Image analysis: Following raw data collection using the software provided by the confocal microscope manufacturer, data stacks were converted to ICS file format (Deanet al. 1990). Custom SCIL-image modules were then used to filter the image stacks, automatically segment the nuclei (Malpicaet al. 1997; Ortizde Solorzanoet al. 1999), and automatically segment the DUMPY (DPY) staining into discrete 3D bodies (Ortizde Solorzanoet al. 1998). A full description of the filters and settings that were used to process the images is available at http://www.genetics.org/supplemental/156/4/1603/DC1. Detailed information about using and obtaining SCIL-image is available at http://www.tpd.tno.nl/TPD/smartsite64.html.

View this table:
TABLE 1

Data summary

Figure 3.

—In many nuclei, one body of DPY staining represents both X chromosomes. (A) A histogram showing that the DPY-27-staining bodies in nuclei containing one body are larger than the DPY-27-staining bodies in nuclei containing two bodies. Overall, the average size of a “disjoined” X was 678 × 106 nm3, about half the volume of a “joined” X (avg. 1338 × 106 nm3). (B) A histogram showing that DPY-27 staining occupies a similar volume regardless of whether the X chromosomes are resolved into one or two bodies. On average, the X occupied 10.2% of nuclear volume (avg. 1338 × 106 nm3) in nuclei with one body and 9.3% of nuclear volume (avg. 1368 × 106 nm3) in nuclei with multiple bodies. The histograms in A and B are derived from wild-type embryos analyzed in experiment 1 of Table 1 (1006 nuclei).

After initial segmentation was complete, images were rendered with daVinci (data visualization and computer interaction; Ortizde Solorzanoet al. 1999). Rendered objects were then scored manually as clusters of multiple nuclei, an individual nucleus, or debris. Rare nuclei that had been inappropriately segmented were rejoined. Objects scored as clusters of nuclei were sent back to SCIL-image and automatically segmented into individual nuclei using a routine based on morphological transformation (distance transform) and the watershed algorithm (Ortizde Solorzanoet al. 1999). Objects scored as debris were not considered for further analysis.

Figure 4.

—Properties of wild-type nuclei and X chromosomes during embryonic development. (A) Average nuclear volume decreases as embryos develop. In both wild-type embryos (solid diamonds, solid line, n = 27) and mnDp10 embryos (open squares, dashed line, n = 22), as cell number increases, the average volume of the nuclei decreases. mnDp10 is a duplication of the right end of X attached to chromosome I (see Figure 5). (B) The volume of the X chromosome decreases with the decrease in nuclear size. All data are from wild-type (N2) embryos (n = 27). Each data point represents an average value from a single embryo. Data from two different antibodies, anti-DPY-26 (n = 14, open squares, dashed line, acquired with a Leica confocal microscope) and anti-DPY-27 (n = 13, solid diamonds, solid line, acquired with a Zeiss confocal microscope) are shown. The DPY-26/Leica experiments consistently produced higher X chromosome volume measurements. Whether this observation is biologically relevant, a property of the particular antibody used, or a property of the microscope that was used has not been determined. Despite the difference in absolute volume observed between DPY-26 and DPY-27 antibodies, the relative decrease in X volume with decreasing nuclear size is similar in the two data sets. (C) As nuclear volume decreases, the X chromosomes appear to occupy a larger percentage of nuclear volume.

For all data sets, objects with a rendered volume of <35 × 106 nm3 were deleted and were not counted in any aspect of the analysis. This cutoff was determined by empirical comparisons of noise in the original confocal data with rendered data and by considering the optical limit of resolution (an object 300 nm × 300 nm × 300 nm = 27 × 106 nm3). The settings for the filters used to render the nuclei and chromosomes were chosen conservatively so that only relatively bright signals with sharp edges would be rendered and counted as objects. For a complete description of how the embryos were analyzed, please refer to the supplemental web site at http://www.genetics.org/supplemental/156/4/1603/DC1.

Sequence analysis: All programs used for sequence analysis and instructions for their use are available at http://www.genetics.org/supplemental/156/4/1603/DC1.

Injections of X-enriched oligo pairs: Extragenic DNA injected into C. elegans forms a heritable, mitotically stable, extrachromosomal mass referred to as an extrachromosomal array. The following oligonucleotide pairs were annealed to form double-stranded DNA and coinjected into worms along with the DNA components of the lacI/lacO system. The resulting extrachromosomal arrays were then assayed for DCC binding activity by staining with antibodies to DCC proteins. The information in parentheses refers to how many repeating units are represented by the oligo:

Clustered repeats:

  1. Left end

    Rpt1 (single unit)

    JDL117 GTTTTGGTCGCTGCTAATTTTTGGTCATTGCTAAT TTTTAGTCAGTGCTAA

    JDL118 TTAGCACTGACTAAAAATTAGCAATGACCAAAAAT TAGCAGCGACCAAAAC

    Rpt2 (single unit)

    JDL119 GGTCAGTGCAACTTAAATTGGTCAGTGCAACTGCA ACT

    JDL120 AGTTGCAGTTGCACTGACCAATTTAAGTTGCACT

    GACC Rpt3 (single unit)

    JDL121 GGTCCGTGCACATGTTTTTTGGTCAGTGCACGTGG TTTCTTTTTCTTT

    JDL122 AAAGAAAAAGAAACCACGTGCACTGACCAAAAAAC ATGTGCACGGACC

    Rpt4 (tandem units)

    JDL123 CAGTGCCTATGAAAGATTGGTCAGTGCCTATGAAA GATTGGT

    JDL124 ACCAATCTTTCATAGGCACTGACCAATCTTTCATA GGCACTG

  2. CeRep27 (not tested)

  3. C07D8 (single unit)

    JDL111 CCGGCGCCCATTTAAGGGTAAGGAATCGCTCTAAG CGAAA

    JDL112 TTTCGCTTAGAGCGATTCCTTACCCTTAAATGGGC GCCGG

  4. Right center (single unit)

    JDL115 AAAACCGCTCCAAAACCGTTCCAATACCGCTCC

    JDL116 GGAGCGGTATTGGAACGGTTTTGGAGCGGTTTT

  5. Short clusters (tandem units)

    JDL125 CGACCTAGGTCGCTAGGTCGCAGGTCGCAAAGCGA CCTAGGTCGCTAGGTCGCAGGTCGCAAAG

    JDL126 CTTTGCGACCTGCGACCTAGCGACCTAGGTCGCTT TGCGACCTGCGACCTAGCGACCTAGGTCG

  6. Right end (single unit)

    JDL113 GAAGTGCTTTCTGTCGTACTCGAAGCAGTGCTGGT GGATGGAGTC

    JDL114 GACTCCATCCACCAGCACTGCTTCGAGTACGACG AAAGCACTTC

    Unclustered repeats: Unclustered #1 (tandem units)

    JDL133 AGGCAGTAACGGTTAGGCAGTAACGGTTAGGCAG TAACGGTT

    JDL134 AACCGTTACTGCCTAACCGTTACTGCCTAACCGT TACTGCCT

    Unclustered #2 (tandem units)

    JDL129 AGGTCACGAGAGGTCACGAGAGGTCACGAG

    JDL130 CTCGTGACCTCTCGTGACCTCTCGTGACCT

    Unclustered #3 (tandem units)

    JDL127 AGTCGGTAGTAGTCGGTAGTAGTCGGTAGT

    JDL128 ACTACCGACTACTACCGACTACTACCGACT

    Unclustered #4 (tandem units)

    JDL131 MGGTCAGTGCGMGGTCAGTGCGMGGTCAGTGCG

    JDL132 CGCACTGACCKCGCACTGACCKCGCACTGACCK

    Unclustered #5 (tandem units)

    JDL137 ACTACGTAAACTACGTAAACTACGTAA

    JDL138 TTACGTAGTTTACGTAGTTTACGTAGT

    Unclustered #6 (tandem units)

    JDL139 CCAGTCGTGCCAGTCGTGCCAGTCGTG

    JDL140 CACGACTGGCACGACTGGCACGACTGG

    Unclustered #7 (tandem units)

    JDL135 TTGCGACCTTTGCGACCTTTGCGACCT

    JDL136 AGGTCGCAAAGGTCGCAAAGGTCGCAA

Raw data: All data that was used in this manuscript can be found and downloaded in tabular form at http://www.genetics.org/supplemental/156/4/1603/DC1.

RESULTS

Three-dimensional reconstructions accurately determine the size and position of nuclei, X chromosomes, and subchromosome-sized objects: The comparisons made in this study are based on the three-dimensional (3-D) reconstruction of X chromosomes or other bodies within the nuclei of individual cells that had been identified by staining with antibodies to the dosage compensation proteins DPY-26 or DPY-27 (referred to as DPY staining). Following confocal microscopy of embryos stained with a DPY antibody and the DNA dye propidium iodide (PI), stacks of images were used to create 3-D reconstructions of the whole embryos, which were then computationally segmented into individual nuclei (materials and methods). This staining and reconstruction procedure allowed us to determine the size and shape of each nucleus and of all the DPY-staining bodies within each nucleus. In wild-type XX embryos, the two X chromosomes can be readily visualized following the 3-D reconstruction of the DPY-staining channel (Figure 2, A-F). By using quantitative data to compare wild-type strains with strains bearing an X chromosome duplication, we sought to detect DCC binding to X chromosome DNA that was attached to an autosome.

Before assaying DCC binding to autosome-attached X duplications, it was necessary to establish that our method was able to detect subchromosome-sized fluorescent signals that were located apart from X and that these signals could be resolved spatially from the X chromosomes. We tested our assay by determining if a small, GFP-labeled extrachromosomal array could be detected and resolved from the X chromosomes in wild-type embryos (materials and methods). Extrachromosomal arrays and the X chromosomes are expected to occupy mutually exclusive positions in the nucleus. XX embryos carrying arrays with lacO operator repeats and gfp-tagged lac repressor genes were fixed and stained with anti-GFP antibody to label arrays, anti-DPY-27 antibody to label the X chromosomes, and DAPI to label all DNA. After confocal microscopy (Figure 2G) and reconstruction (Figure 2, H and I), the arrays were easily detected. On average, each array occupied 1.79% of the nuclear volume and had an average volume of 337 × 106 nm3, about half the volume of a single X chromosome (see below). Our ability to resolve the X chromosomes and the arrays in three-dimensional space inside of C. elegans nuclei is important because it suggests that DPY staining located apart from X could be resolved spatially from the X chromosomes. Therefore, if the DCC were bound to a partial X-chromosome duplication attached to an autosome, the binding could be detected by our staining and reconstruction procedure.

Figure 5.

—The strategy and tools for examining X chromosome duplications. (A) A map of selected X chromosome duplications. The name of the duplication is in italics, followed by its chromosomal attachment point (f = free), the number of genetic map units (mu) covered, and the approximate percentage of the X chromosome covered. Percentages may be overestimates, since coverage is defined genetically and some duplications contain uncharacterized internal deletions. mnDp10 is known to have large deletions left of unc-9 (map position 11.6): unc-58 (1.50) and unc-115 (1.7) are covered by mnDp10, but dpy-22 (1.99), vab-3 (2.01), and lin-14 (3.48) are not. Although the precise extent of the deletions is not known, we estimate that mnDp10 covers ∼30% of X on the basis of the available map data. Duplications in black were tested for DCC binding activity in this study. (B) A schematic representation of a wild-type karyotype and an mnDp10 karyotype.

Properties of wild-type nuclei and X chromosomes during embryonic development: We determined the general morphological properties of X chromosomes in wild-type embryos to establish a firm baseline for comparison to X-duplication-bearing embryos. Although all cells of the embryos used in this analysis contained two X chromosomes, two separate DPY-staining bodies were observed in only 31.6% of nuclei, while one staining body was observed in 63.6% of nuclei (Table 1). To examine the reason for the disparity between the known and observed number of X chromosomes, nuclei with only one recorded staining body were reviewed manually. In many of these nuclei, two DPY-staining bodies were discernible, but were counted as only one by the computer software because the two bodies were separated by a distance less than our limit of resolution or were connected by a “bridge” of fluorescence (Figure 2J). To confirm that X chromosome proximity interfered with the quantitation, comparison was made between total X chromosome volume in nuclei recorded as containing one DPY-staining body (referred to as a “joined” X) and the volume of each of the DPY-staining bodies in nuclei recorded as having two X’s (referred to as an “disjoined” X). If the joined X chromosomes truly represent two X’s, then the volume of joined bodies should be approximately twice that of each of the individual disjoined bodies. If the joined class of staining bodies represents only one X, then the volumes of the two classes should be roughly equal. We found that the average volume of a DPY-staining body in nuclei with one object is 1338 × 106 nm3 (±18 × 106, standard error) and in nuclei with two objects is 678 × 106 nm3 (±17 × 106, standard error, Figure 3A). These results indicate that nuclei recorded as having one object actually contain two X chromosomes, as expected. This conclusion is confirmed by the observation that DPY staining occupies a similar total volume in nuclei that contain one staining body as in nuclei that contain two staining bodies (Figure 3B). The failure to resolve the two X chromosomes in nearly two-thirds of wild-type nuclei is important to consider when interpreting results from duplication strains.

Another expectation is that more than two bodies of DPY staining should never be visible in the nuclei of wild-type embryos. However, in wild-type nuclei, three bodies of staining were observed 4.2% of the time, and four bodies in 0.5% of nuclei. These rare nuclei may contain an X chromosome with a weakly staining region that causes it to be counted as two separate bodies or a spurious antibody signal that creates an artifactual object. Possibly, a small fraction of nuclei were captured in early anaphase of mitosis and therefore do contain more than two discernible X chromosomes.

Figure 6.

mnDp10 embryos have more individual DPY-staining bodies per nucleus than wild-type embryos, and total DPY staining occupies a greater percentage of the nuclear volume. (A-C) Number of DPY-staining bodies per nucleus compared in wild-type (black) and mnDp10 (red) nuclei. (D and E) Volume of DPY-staining bodies compared in mnDp10 and wild-type nuclei. These histograms show the percentage of nuclear volume occupied by DPY staining on the x-axis, with the percentage nuclei containing that volume of staining on the y-axis. The distribution of mnDp10 nuclei shows a pronounced shift to the right, indicating an increase in total DPY-27 staining. In D, this difference occurs despite a higher average age for wild-type embryos (135 cells) compared to mnDp10 embryos (114 cells). For E, average ages were 161 cells for wild-type embryos and 171 cells for mnDp10 embryos.

Finally, it was essential to ensure that our analysis was not skewed by differences in nuclear or chromosomal architecture that may occur throughout embryonic development. Therefore, we determined how nuclear volume and X chromosome volume varied with each other and how they varied with embryonic age. We expected that nuclear volume, as determined by PI staining, would decrease as the embryos aged because the size of the chitinous egg shell remains constant throughout embryonic development, while the embryo’s cell number increases from 1 to 558. As expected, we observed that the average nuclear volume decreases as embryos develop (Figure 4A, age range 26-368 cells). One might also expect the volume of X chromosomes to shrink proportionally with the decrease in nuclear volume. We found that the volume of the X chromosomes does vary with nuclear size (Figure 4B), but as nuclear volume decreases, the volume of the X chromosomes appears to decrease at a slower rate (Figure 4C). Therefore, although the X chromosomes get smaller as nuclei get smaller, they appear to occupy a larger proportion of the nucleus as nuclear volume decreases. Although the reason for this phenomenon is not known, its effects are averted in all analyses in two ways. First, embryos are compared only if they are approximately age matched, and second, the percentage of nuclear volume occupied by DPY staining is expressed as a function of nuclear volume where appropriate. The effect could be caused by the fact that volume measurements become less accurate, and are more likely to be overestimated, as the size of an object decreases. Thus, smaller objects are subjected to a proportionally larger error in measurement than bigger objects. In addition, the different staining methods may affect the relative accuracy of measurements to different degrees, depending on the object size.

Figure 7.

—In mnDp10 embryos, DPY-staining occupies a greater percentage of the nuclear volume, regardless of nuclear size. (A) The average percentage of nuclear volume occupied by DPY-26 staining is plotted against average nuclear volume for mnDp10 embryos (n = 10) and wild-type embryos (n = 14). Each data point represents the average values for a single embryo. (B) Same as for A, but with anti-DPY-27-stained mnDp10 embryos (n = 13) and wild-type embryos (n = 13).

The DCC recognizes and associates with the X duplication mnDp10 but apparently does not spread onto adjacent autosomal regions: To determine if the dosage compensation complex recognizes and associates with subregions of the X chromosome, we compared the distribution of DPY staining in wild-type XX embryos and XX embryos that also contain two copies of an autosome-attached X duplication. We first assayed embryos carrying mnDp10, a duplication of the right ∼30% of the X chromosome attached to the right end of chromosome I (Hermanet al. 1979; Figure 5).

We envisioned three possible outcomes in comparing mnDp10-bearing and wild-type embryos (Figure 5B). The first outcome is that the DCC can bind the duplication and that the DPY-staining associated with the duplication can be resolved spatially from the X chromosomes. The second outcome is that the DCC can bind the duplication, but for technical or biological reasons cannot be resolved spatially from the X. The final outcome is that the DCC is unable to bind the duplication, or we are unable to detect the binding. Two independent questions were asked to distinguish these outcomes: (1) Is there an increase in the number of DPY-staining bodies per nucleus in duplication-bearing strains? (2) Does total DPY staining occupy a larger portion of the nuclear volume in duplication-bearing strains? The first outcome demands an affirmative answer to both questions and would indicate that the autosome-attached duplication can be recognized as X chromosome DNA. The second outcome predicts a negative answer to question one, but an affirmative answer to question two. Finally, a negative answer to both questions would indicate either that the duplication cannot be recognized as X chromosome DNA or that its size or brightness is below the physical limits of detection.

If the DCC binds the duplication and can be resolved from the X chromosomes, a third question would be asked to address whether the duplication acts as a nucleation center for DCC binding, which then spreads onto autosomal sequences: Is there a new class of DPY-staining bodies in duplication-bearing strains, and how large are these new bodies compared to a normal X? If the new DPY-staining bodies are large (chromosome-sized) then the duplication may act as a nucleation center for DCC binding, with subsequent spreading into autosomal sequences. If the extra staining bodies are small (duplication-sized), then it is likely that only the duplication is recognized as X and that the binding does not spread a significant distance onto autosomal DNA.

The number of DPY-staining bodies is increased per nucleus in mnDp10-bearing strains: The three histograms shown in Figure 6, A-C, each representing an independent experiment, reveal a consistent increase in the number of DPY-staining bodies per nucleus in mnDp10 strains. In each of the three experiments, a lower proportion of the mnDp10 nuclei contain one staining body (53, 51, and 49%) compared to wild-type nuclei (66, 62, and 63%, respectively). This difference exists because a higher proportion of mnDp10 nuclei contain two (34, 41, and 38%) or three (12, 8, and 10%) DPY-staining bodies compared to wild-type nuclei (two bodies: 30, 33, and 33%; three bodies: 0.3, 0.3, and 0.4%). These results suggest that DPY-27 and DPY-26 localize to mnDp10 and that this localization is manifested by the appearance of extra staining bodies. One might expect to see four DPY-staining bodies in nuclei that harbor an X duplication (the two X’s and the two duplications). However, the appearance of any extra bodies would be obscured by the same factors that cause 65% of wild-type XX nuclei to be counted as having one body of DPY staining. Furthermore, any additional DPY staining in the nuclei of mnDp10 strains would further crowd the nucleus with fluorescence signal, making it even more difficult to resolve the additional mnDp10 bodies. Considering these confounding factors, we interpret the consistently observed changes in the proportion of nuclei harboring multiple staining bodies to be significant. Therefore, an increase in the number of DPY-staining bodies per nucleus is observed in mnDp10-bearing embryos compared to wild-type embryos, consistent with a new, physically distinct target for the DCC.

Figure 8.

—A new class of small DPY-staining bodies is present in mnDp10 embryos. In each of the three histograms, the percentage of nuclear volume occupied by individual DPY-staining bodies is plotted on the x-axis for both wild-type (black) and mnDp10 (red) nuclei. The y-axis shows the percentage of all nuclei that contain a body of the size indicated on the x-axis. In mnDp10 strains, there is a marked increase in the number of staining bodies that occupy < ∼2.5% of nuclear volume.

Total DPY staining occupies a larger portion of the nuclear volume in mnDp10-bearing strains: If mnDp10 is recognized by the dosage compensation complex, one would expect an increase in the total amount of DPY staining in each nucleus. Assuming that mnDp10 is 30% of X, one would ideally expect DPY staining to occupy an additional ∼3% of nuclear volume. In mnDp10 strains, DPY-27 staining (experiments 1 and 2, Table 1) occupied an additional 0.90% of the nuclear volume (wild type, 10.06 ± 0.08% standard error; mnDp10, 10.96 ± 0.10%), representing an 8.9% increase (P = 1.45 × 10-12, two-tailed Student’s t-test) compared to the expected 30%. In agreement with this increase, total DPY-26 staining (experiments 3 and 4, Table 1) occupies an additional 1.05% of nuclear volume in mnDp10 strains (wild type, 14.11 ± 0.09%; mnDp10, 15.15 ± 0.13%), an increase of 7.4% (P = 2.05 × 10-11, t-test). This increase in total staining is reflected in the histograms shown in Figure 6, D and E. These charts show the percentage of nuclear volume occupied by DPY staining (x-axis) plotted against the percentage of nuclei containing that volume of staining (y-axis). The distribution for mnDp10 nuclei is shifted to the right, indicating an increase in total DPY-27 staining. For example, in Figure 6D every bin to the right of 12% contains more mnDp10 nuclei, while every bin to the left of 12% contains more wild-type nuclei. The deviation from the ideal increase (∼30%) in staining probably reflects the challenge of resolving mnDp10 from the X chromosome in crowded nuclei (see also below).

The observed increase in the percentage of volume occupied is not a consequence of age differences between mnDp10 embryos (average age, 139 cells) and wild-type embryos (average age, 154 cells), since for both DPY-26 and DPY-27 antibodies, mnDp10 strains exhibit an increase in DPY-staining volume regardless of nuclear volume. This result is shown in Figure 7, where the percentage of nuclear volume occupied by DPY staining was plotted as a function of nuclear volume. The demonstrated increase in DPY staining in mnDp10 nuclei indicates that the additional DPY-staining bodies found in mnDp10 embryos arise from new target sequences, rather than from a physical reorganization of existing targets. Furthermore, the magnitude of the increase (∼8%) suggests that mnDp10 is represented by an additional small body of staining.

A new class of small DPY-staining bodies exists in mnDp10-bearing strains: To test the hypothesis that mnDp10 is represented by an additional small body of DPY staining, we recorded the volume occupied by individual DPY-staining bodies in wild-type and mnDp10 nuclei. We then calculated the percentage of nuclear volume occupied by individual DPY-staining bodies. Histograms of the data (Figure 8) show a dramatic increase in the occurrence of small DPY-staining bodies in the mnDp10 strain. We interpret the new class of DPY-staining bodies to be mnDp10. Such a body can be visualized in the 3-D reconstruction shown in Figure 9.

We used the data from Experiment 1 (Figure 8) to determine the properties of the new class of DPY-staining bodies. If mnDp10 is defined conservatively as bodies occupying 0.2-2.2% of nuclear volume, an mnDp10-sized body was found in an average of 34.1% of mnDp10 nuclei, compared to 13.0% of N2 nuclei, a 2.6-fold increase. On the basis of the appearance of the new class of DPY-staining bodies, mnDp10 may also be defined in absolute terms as DPY-staining bodies ranging in volume from 35-400 × 106 nm3. To ascertain how reliably we could score the presence of mnDp10, we asked how often we could detect a joined X [defined as >(1337 × 106 nm3 - 1 SD)] plus mnDp10 (defined as a body of size 35-400 × 106 nm3) or two X chromosomes (both 678 × 106 nm3 ± 1 SD) plus mnDp10. These conditions were satisfied in 27.1% of mnDp10 nuclei and only 12.1% of N2 nuclei. Therefore, using these empirical definitions, we are able to detect the two X chromosomes and mnDp10 in 27% of all mnDp10 embryonic nuclei, with a false positive rate of 12%.

Figure 9.

—Visualization of mnDp10. (A-C) Surface rendering of a nucleus containing mnDp10 stained with propidium iodide (light blue) and anti-DPY-27 antibody (dark blue). The X points to the X chromosomes, and the D points to the small piece of DPY-27 staining that we interpret to be mnDp10. Overall, it is estimated that both X chromosomes and an mnDp10 staining body can be identified in 27% of all mnDp10 nuclei (see text for explanation). The black plane shows an individual section of the original confocal data from the anti-DPY-27 channel.

This low level of detection may be due to the crowding of fluorescence in the nucleus. In fact, this problem would be compounded by any additional DPY staining caused by mnDp10, making it likely that many mnDp10 bodies are not resolved from each other or from the normal X chromosome staining. A biological explanation may also exist: perhaps mnDp10 is only recognized by the DCC a certain percentage of the time or is recognized only in particular tissues. These factors, along with physical limits on the resolution of light microscopy and the small size of C. elegans nuclei (materials and methods), conspire to make the detection of an extra staining body difficult, especially without an independent marker for the position of the duplication in the nucleus.

In nuclei interpreted to contain mnDp10, the DPY staining that defines the duplication occupies an average of 1.06% of total nuclear volume, or 182 × 106 nm3. For comparison, the average volume of a single X is 678 × 106 nm3, indicating that mnDp10 occupies on average 26.76% of the volume of a single X (data from experiment 1, Table 1). Therefore, new DPY-staining bodies observed in the mnDp10 strains occupy a small volume compared to the volume of the X chromosome, a result consistent with the dosage compensation machinery binding to X sequences but not spreading far onto adjacent autosomal sequences, if at all. This result demonstrates that the duplication contains all the information necessary to specify X identity and that the dosage compensation machinery can localize to a site distinct from the normal X chromosomes. However, this result does not rule out a spreading mechanism. Should spreading from a nucleation center be the means by which complexes extend along X, an X duplication must attach to an autosomal location that would block the spreading; otherwise, the X duplication would cause reduced autosomal gene expression and probably death. Nonetheless, the absence of extensive spreading does support the hypothesis that a more evenly distributed X recognition signal is required for the propagation of DCC binding.

yDp14, stDp2, and mnDp27 embryos are indistinguishable from wild-type embryos: To examine other areas of the X chromosome for DCC-binding activity, we analyzed strains carrying either yDp14, a duplication of the left end of X that is also attached to chromosome I; stDp2, a duplication of the center of X integrated into chromosome II; or mnDp27, a duplication of the right end of X attached to the end of chromosome II (Figure 5).

To analyze yDp14, a total of 1759 nuclei from 10 embryos were examined (Table 1 and web supplement) using the same experimental tests and filtering conditions that were applied to the mnDp10 embryos. Unlike mnDp10 embryos, yDp14 embryos showed no significant increase in the number of DPY-27 staining bodies per nucleus (Figure 10A, Table 1). Overall, the same proportion of yDp14 nuclei contained one (66%), two (31%), and three (3%) bodies of staining as wild-type nuclei (64, 32, and 4%, respectively). In addition, no consistent increase in total DPY-staining volume was observed (Figure 10, B and D). Finally, no new class of DPY-staining objects appeared in yDp14 strains (Figure 10C). When the same analysis was applied to 3134 stDp2 nuclei and 1374 mnDp27 nuclei (Table 1 and web supplement), no significant deviation was seen from wild-type nuclei for any of the three aspects of staining that were measured. These results indicate that either the DCC cannot recognize yDp14, stDp2, and mnDp27 as X chromosome DNA or that the size and intensity of the signal produced by the binding of the duplication falls below the limit of detection for this method.

Figure 10.

—DPY staining in yDp14 nuclei is not significantly different from DPY staining in wild-type nuclei. (A) No increase is found in the number of DPY-staining bodies in yDp 14 embryos. On average, yDp14 nuclei contained 1.37 bodies per nucleus, compared to 1.42 bodies per nucleus for wild-type and 1.63 for mnDp10 embryos. (B) DPY staining occupies a similar volume in wild-type and yDp14 embryos. (C) No new class of DPY-staining bodies exists in yDp14 embryos. (D) No increase is observed in the proportion of the nuclear volume occupied in yDp14 strains, regardless of nuclear volume. The average percentage of nuclear volume occupied by DPY staining is plotted against average nuclear volume for yDp14 embryos (open squares, dashed line) and wild-type embryos (solid diamonds, solid line). Each data point represents the average values for a single embryo. Unlike mnDp10 embryos (Figure 7), the trend line calculated for these duplication-bearing embryos is very close to the trend line for wild-type embryos. All data shown in this figure are from experiment 3. These data are representative of the negative results observed for stDp2 and mnDp27 (for data, see http://www.genetics.org/supplemental/156/4/1603/DC1).

X chromosome DNA has 14 families of X-enriched sequence elements: In mnDp10 embryos, the failure of the DCC to spread from X sequences to autosomal sequences suggests that C. elegans X recognition elements may be widely distributed across the X. Therefore, spreading might not have to occur over large distances. To identify potential X recognition elements, we analyzed the C. elegans genome sequence (99% complete) using a computational approach. Our goal was to identify repeated X-enriched sequence strings that may act as X recognition elements. We wrote a program called “count” that can determine the frequency of every string of length N that occurs on a chromosome, where N is any number supplied by the user. To find X-enriched sequences, we used this program to look for nonamers that occur >75 times on X and occur at least 10 times more frequently on X than on the autosomes (Table 2; see materials and methods for details). The 58 nonamers that meet these criteria are listed in Table 2. A string length of nine was found to produce the most informative results. Shorter strings occur too often by chance (they are “noisy”), and we found that 9-bp queries were able to detect much longer repeat units, since units >9 bp will also contain a repeating unit of 9 bp.

View this table:
TABLE 2

Nonamers that occur >75 times on X and are at least 10-fold X enriched

View this table:
TABLE 3

Repeat families derived from X-enriched 9mers

To determine which of the nonamers were members of a common family of X-enriched elements, we wrote a program that maps the position of strings onto any sequence file (materials and methods). We reasoned that strings representing the same repeating unit could be sorted into families by determining which of them have similar distribution patterns. By comparing the distribution patterns of the 58 selected strings, 14 families of X-enriched sequences were identified (Table 3). We found that these 14 families could be further divided into one group of six, whose repeat elements were concentrated in tight clusters on the X chromosome (Figure 11), and one group of eight, whose repeated elements were more evenly dispersed across the X (Figure 12). The distribution patterns of the X-enriched sequence families are diverse, ranging from the majority of occurrences on a single cosmid to a roughly even spacing along the X chromosome. By manual inspection, the true repeating unit of each of the families was found to range from 32 to 226 bp (Table 3). The mnDp10 results suggest that X-enriched sequence families that occur in a very confined region of X are less likely to be X recognition elements. The remaining “unclustered” candidate X recognition sequences provide a solid starting point for further dissection of the cis-acting elements that determine the binding specificity of the dosage compensation complex.

To test the biological significance of the X-enriched repeats, complementary oligonucleotides specific for the repeating unit of each family were synthesized, the oligos were annealed to form duplex DNA, and the resulting double-stranded DNAs were assayed for DCC binding activity in the lacI/lacO array-based system (materials and methods; Daweset al. 1999). Of the 15 oligonucleotide pairs tested for activity, all gave a negative result. Future experiments will examine each of the repeat sequences in the context of larger segments of X DNA to determine whether they are necessary, but just not sufficient, to recruit the dosage compensation machinery.

Figure 11.

—The X chromosome distribution of clustered X-enriched motifs. The positions of a representative member of each family of clustered X-enriched sequences are shown as a histogram. Numbers on the x-axis represent the location in base pairs (×105). Bars represent number of occurrences in each 10,000-bp bin. The actual sequence mapped for each sequence family are underlined in Table 2.

DISCUSSION

Our work leads to important conclusions regarding the mechanism used by the dosage compensation machinery of C. elegans to recognize X chromosomes. We have shown that the dosage compensation machinery can assemble on a site distinct from the full-length X chromosome, namely, on a partial duplication of X that has been removed from its normal chromosomal context through its linkage to an autosome. Therefore, a discrete portion of X can retain its identity as X and its ability to recruit the dosage compensation machinery. In our experiments, the dosage compensation machinery appears not to have spread far, if at all, onto adjacent autosomal sequences. The lack of significant spreading suggests that X chromosome recognition and DCC binding in C. elegans may not proceed via the mechanism used by mammals to inactivate their X chromosome: nucleation and spreading from a single site. It is more likely that either no spreading occurs in C. elegans or that limited spreading occurs from several chromatin entry sites, as proposed for Drosophila. However, in view of the caveats discussed below, it remains possible that the X chromosome contains a single site for binding the DCC complex, and the transcriptional repression spreads from there.

Figure 12.

—The X chromosome distribution of unclustered X-enriched motifs. The positions of a representative member of each family of unclustered X-enriched sequences are shown as a histogram. Numbers on the x-axis represent the location in base pairs (×105). Bars represent number of occurrences in each 10,000-bp bin. The actual sequences mapped for each sequence family are underlined in Table 2.

The initial suggestion that X chromosome duplications might compete with the normal X chromosome for dosage compensation proteins came over 12 years ago with a study showing that X chromosome duplications affect the expression of X-linked genes that were not duplicated (Meneely and Nordstrom 1988). In that study, the phenotype caused by an X-linked hypomorphic lin-15 mutation was partially suppressed by mnDp25 and stDp2, suggesting that expression of lin-15 could be increased without increasing its gene copy number. This conclusion was corroborated by an assay that demonstrated an increase in the enzymatic activity of the X-linked acetylcholinesterase gene ace-1, also not duplicated by mnDp25 or stDp2. mnDp10 was not examined because it covers both loci. However, in a separate study using Northern blots as a direct measure of gene activity, mnDp10 was shown to increase the mRNA levels of uvt-4 and uxt-1, two X-linked loci not duplicated by mnDp10 (B. J. Meyer, unpublished data).

Both sets of experiments were conducted before the discovery of the dosage compensation complex, and it was not possible then to distinguish between two competing hypotheses. The first hypothesis was that the duplications titrated a repressor of gene expression away from X, while the second contended that the duplications contained wild-type copies of one or more general enhancers of X-linked gene expression or, less likely, enhancers of the specific loci tested. Increased gene expression might also have arisen from other physiological perturbations caused by the duplication. Experiments have since shown that the DCC binds to X (Chuang et al. 1994, 1996; Lieb et al. 1996, 1998), but whether the DCC is capable of binding to X chromosome duplications has not been determined. Therefore, the results presented here permit us to interpret the previous duplication experiments in a new light and to conclude that the repressive dosage compensation machinery can be titrated away from X by a duplication. The combination of results also implies that at least one DCC component is limiting for full dosage compensation function.

Do X chromosome duplications make good models for the behavior of X chromosomes during dosage compensation? Valid concerns temper the conclusions that can be made on the basis of the DCC-binding properties of mnDp10. Any duplication that could act as a nucleation site for the spreading of the DCC onto an autosome would be expected to cause hermaphrodite lethality. Presumably, such duplications would be selected against during the isolation procedure, and therefore only duplications that fail to act as centers for nucleation and spreading would have arisen. This concern is heightened by the unusual number of duplications attached to the right end of chromosome I, suggesting that some selection for that attachment point occurred. One possibility is that the presence of the 28S rDNA repeat cluster at the right end of chromosome I might preclude spreading and therefore select for the attachment of X duplications adjacent to it.

These caveats are difficult to address directly. Unfortunately, for the analysis presented here, it was essential that the partial X duplications be physically attached to an autosome, because unattached duplications are not mitotically stable, and their loss during embryonic development is difficult to monitor. In addition, only strains that are viable as duplication homozygotes are amenable to analysis because no practical way exists in our assay to distinguish among embryos with zero, one, or two copies of the duplication. These restrictions sharply reduce the number of duplications available for study. Furthermore, chromosomal duplications are created essentially at random by irradiation, making it difficult to create “custom” duplications or attachment points. Two of the duplications analyzed in this study, stDp2 and mnDp27, were chosen because they are not attached to chromosome I and do not cause lethality when homozygosed. However, both duplications produced negative results.

These negative results may be due to the biological inability of the DCC to bind these duplications or to the technical limitations of our assay system. When interpreting the negative results, it is important to consider the positive case, mnDp10. For mnDp10 strains, we estimated that only one in four nuclei contained an independent DPY-staining body that could be scored as mnDp10, and this number drops to only 15% if false positives are subtracted. mnDp10 is the largest of the X duplications examined, and it stands to reason that smaller duplications might be detected less frequently by our assay. Therefore, negative results do not rule out the possibility that the DCC can bind to the duplications in vivo.

The work presented here provides a solid foundation for addressing important unanswered questions regarding the mechanism of X chromosome recognition in C. elegans. A pressing challenge is to determine the precise nature of the DNA elements that specify X chromosome identity. In principle, the features that distinguish X chromosomes from autosomes might include specific repeated X-DNA sequences or X-specific DNA structures. Alternatively, instead of recruitment factors on X, repelling factors might exist on autosomes to prevent the dosage compensation machinery from binding. Although our experiments do not discriminate among these possibilities, they do indicate that the DCC can assemble on X DNA sequences removed from the context of the entire X chromosome, implying that further investigations using the GFP-tagged artificial-chromosome assay to delineate candidate X recognition sequences may prove fruitful.

Important leads in the search for X recognition elements may also emerge from the 14 families of X-enriched sequence elements that were discovered and mapped onto the X chromosome. The similarity between C. elegans dosage compensation proteins and general mitotic factors in worms and other organisms suggests that understanding further how X is distinguished from the autosomes in C. elegans will reveal fundamental properties of chromatin recognition by more general factors.

Acknowledgments

We thank Aaron Straight for providing the lacO repeat plasmid pSV2-dhFr8.32 used in the array studies and Aidyl Gonzalez-Serricchio for providing plasmid pPD49-78, which expresses lacI-gfp under the control of the hsp-16 heat-shock promoter. We are grateful to Donna Albertson for advice concerning microscopy and to Stuart Scherer for advice concerning the analysis of X-enriched repeats.

Footnotes

  • Communicating editor: R. K. Herman

  • Received July 7, 2000.
  • Accepted August 14, 2000.

LITERATURE CITED

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