The Perinucleolar Compartment and Transcription

HeLa cells were grown to subconfluence on 22 × 22-mm glass coverslips in 35-mm Petri dishes in Dulbecco's modified Eagle's minimum essential medium (DMEM) supplemented with 10% fetal calf serum (FCS) (GIBCO-BRL, Life Technologies, Inc., Rockville, MD). The inhibition of RNA polymerase I transcription was achieved by the addition of actinomycin D (0.04 μg/ml for 3 h) (Perry, 1963). The inhibition of RNA polymerase II transcription was achieved by the addition of α-amanitin (50 μg/ ml for 5 h) (Kedinger et al., 1970; Lindell et al., 1970) or 5,6-dichloro-1-β-d-ribofuranosylbenzimidazole (DRB) (25 μg/ml for 3 h) (Sehgal et al., 1976) to the culture medium. Transcription inhibition was reversed when DRB-containing medium was removed from cells and replaced with fresh medium. Cycloheximide (Sigma Chemical Co., St. Louis, MO) was added at 100 μg/ml for 5 h to inhibit protein synthesis and RNA polymerase I activity (Higashi et al., 1968; Willems et al., 1969; O'Keefe et al., 1994).

Transiently expressed GFP–PTB (Huang et al., 1997) was used as a marker to indicate the localization of the PNC. The corresponding nuclear region identified by fluorescence of the GFP–PTB fusion protein was examined by electron microscopy. Specifically, transfected cells were seeded onto gridded glass coverslips. 12 h after transfection, cells were fixed in 4% paraformaldehyde with 0.05% glutaraldehyde in PBS, and cells that showed the PNC were quickly photographed using an epifluorescence microscope (model FXA; Nikon, Inc., Melville, NY) equipped with a cooled CCD camera (1320 × 1035, 6.7 μm pixel size) (SenSys; Photometrics, Inc., Tuscon, AZ) using Oncor Image software. Subsequently, cells were fixed in 2% glutaraldehyde for 20 min and washed in PBS and 0.1 M cacodylate buffer, pH 7.4. Cells were then postfixed in 1% osmium tetroxide containing 0.15% ferrous cyanide in 0.1 M cacodylate buffer, pH 7.4, for 1 h, dehydrated by incubation in a series of ascending concentrations of ethanol, and embedded in Epon/araldite at 60°C for 48 h. Serial 80-nm-thick sections were poststained with uranyl acetate–lead citrate, mounted on slot grids, and examined at 80 keV with a transmission electron microscope (model 100CX; JEOL U.S.A., Inc., Peabody, MA). The same cells photographed at the fluorescence microscopic level were located, and serial images of the nuclear regions that corresponded to the PNCs were recorded. Outlines of the nucleoli and PNCs were hand traced on 11” × 14” photographic prints and digitized using a digitizing tablet and a software program described by Young et al. (1987). The section planes were aligned, and volumes were surface-rendered using the programs SYNU and SYNU-render as previously described by Hessler et al. (1992).

Cells were extracted following a modification of a protocol described by Fey et al. (1986). Subconfluent cells grown on glass coverslips were rinsed with PBS and incubated at 4°C for 10 min in CSK buffer (100 mM NaCl, 300 mM sucrose, 10 mM Pipes, pH 6.8, 3 mM MgCl₂, 1 mM PMSF, and 2 mM vanadyl ribonucleoside complex) containing 0.5% Triton X-100 (vol/ vol). Cells were incubated at 4°C for 5 min in the CSK buffer containing 250 mM ammonium sulfate and 0.5% Triton X-100, treated with DNAse I in CSK buffer with 50 mM NaCl for 30 min at 37°C or room temperature, and finally fixed in 2% paraformaldehyde in PBS.

Expression constructs were transiently transfected into HeLa cells by electroporation (Spector et al., 1997). Subconfluent cells in a 100-mm culture dish were trypsinized and collected in DMEM supplemented with 10% FBS. Cells were then mixed with 20 μg of DNA including 7 μg target DNA and 13 μg sheared salmon sperm DNA. 280 μl of cell–DNA mixture was electroporated in a Bio-Rad electroporator (Hercules, CA) at 260 V and 960 μF. Cells were subsequently seeded onto glass coverslips in 35-mm Petri dishes and were grown for either 7 or 24 h.

Living cell studies were performed using a 35-mm Petri dish with a coverslip attached to the bottom. Transfected cells were grown on the coverslip for 24 h and observed using an inverted confocal laser-scanning microscope (model 410; Carl Zeiss, Inc., Thornwood, NY). An initial image was acquired, and a FRAP macro was used to photobleach a designated area of the nucleus. The photobleaching was accomplished using the 488-nm argon laser at 50% of its full power (25 mW) for 20 s. Immediately after the bleaching process, an averaged image was obtained. Multiple images were subsequently acquired within 5 min after bleaching, as indicated in Fig. 6.

The transcription assay was modified from published studies (Jackson et al., 1993; Wansink et al., 1993). At 8 or 24 h after transfection, cells were rinsed once with PBS and once with a Tris-glycerol buffer (20 mM Tris-HCl, pH 7.4, 5 mM MgCl₂, 25% glycerol, 0.5 mM PMSF, and 0.5 mM EGTA). Cells were then permeabilized in the same buffer containing 5 μg/ml digitonin at room temperature for 3 min. Subsequently, cells were incubated in transcription cocktail (100 mM KCl, 50 mM Tris-HCl, pH 7.4, 5 mM MgCl₂, 0.5 mM EGTA, 25% glycerol, 1 mM PMSF, 2 mM ATP, 0.5 mM CTP, 0.5 mM GTP, 0.2 mM Breakup or 0.4 mM FITC-CTP, and 1 U/ml RNasin) for 5 min at 37°C. At the end of the transcription reaction, cells were gently rinsed three times with PBS and then fixed in 2% formaldehyde in PBS. Transcription inhibition was achieved by adding the corresponding drugs to the permeabilization buffer and transcription cocktail.

Subconfluent HeLa cells grown on glass coverslips were extracted with CSK buffer containing 0.3% Triton X-100 for 3 min and fixed in freshly made 2% formaldehyde in PBS for 15 min. Cells were washed three times for 10 min each in PBS, and coverslips were incubated with primary antibody for 1 h at room temperature. Antibodies used in this study included anti-PTB primary antibody, SH54 (Huang et al., 1997), at a dilution of 1:300, anti-Sm antibody (Lerner and Steitz, 1979) at a dilution of 1:1,000, anti-B″ at a dilution of 1:10 (Habets et al., 1987, 1989), antifibrillarin (Sigma Chemical Co.) (Ochs et al., 1985) at a dilution of 1:5, anti-SC35 at a dilution of 1:1,000 (Fu and Maniatis, 1990), anti–PAB II at a dilution of 1:10 (Krause et al., 1994), or anticoilin at a dilution of 1:100 (Andrade et al., 1993). Cells were rinsed in PBS, incubated with Texas red–conjugated goat anti–human, FITC- or Texas red–conjugated goat anti–mouse, or Texas red goat anti–rabbit antibody at a dilution of 1:100 for 1 h at room temperature, and then washed three times for 10 min each in PBS. The coverslips were mounted onto glass slides with mounting medium containing 90% glycerol in PBS with 1 mg/ml paraphenylenediamine as an antifade agent. The mounting medium was adjusted to pH 8.0 with 0.2 M bicarbonate buffer (Spector et al., 1997). Cells were examined with a microscope (model FXA; Nikon, Inc.) equipped with epifluorescence and differential interference contrast optics. Images were captured by a cooled CCD camera (1320 × 1035, 6.7 μm pixel size) (SenSys; Photometrics, Inc.) using Oncor Image software.

Previous examination of thin-sectioned and optimally fixed HeLa cells revealed that the PNC is an electron-dense structure composed of thick strands, some of which are in direct contact with the surface of the nucleolus (Huang et al., 1997). We sought to determine if these thick strands are interconnected and if they form a higher order structure. To resolve the three-dimensional organization of the PNC at high resolution, PNCs in serial thin sections of optimally fixed HeLa cell nuclei were examined by electron microscopy (Materials and Methods). The sections were poststained with uranyl acetate–lead citrate, and the PNC was readily distinguishable from the nucleolus under these conditions of specimen preparation. The PNC was also identified by correlating the cell sections to a fluorescent image of the same cell in which the expression of GFP–PTB (Huang et al., 1997) marked the PNC (Fig. 1). The PNC appeared to be more electron dense than the nucleolus and formed thick strands, some of which intimately associate with the nucleolus. Images of serial sections were aligned, and three-dimensional models were reconstructed using the programs SYNU and SynuRender (Hessler et al., 1992) (Fig. 2). Such analysis has revealed that the PNC is a highly interconnected and reticulated mesh associated with a portion of the nucleolar surface. However, there is considerable variability in the shape, size, and the relationship of the PNC with the nucleolus. In some cells, the PNC is mostly positioned on the surface of the nucleolus (Fig. 2,A), while in others, the PNC extends into the nucleolus like a plug (Fig. 2,B). Occasionally, a portion of the nucleolus extends into the PNC (Fig. 2 C). This variability may represent the dynamic range of PNC:nucleolus interrelationships.

Based on the abundance of RNAs and RNA-binding proteins in the PNC, we were interested in examining if this subnuclear compartment is involved in transcription. In situ Br-UTP incorporation experiments were performed to evaluate the transcriptional activity in the PNC. Cells transiently expressing GFP–PTB, which marks the PNC, were briefly permeabilized and incubated in a transcription cocktail containing Br-UTP using a modified protocol based on the work of Wansink et al. (1993) and Jackson et al. (1993). Cells were then fixed, and the nuclear sites of Br-UTP incorporation were detected by immunolabeling with a monoclonal antibody that specifically recognizes the Br epitope. Simultaneous detection of the incorporation sites (red signal) and the PNC, marked by GFP–PTB (green signal), demonstrates that the PNC coincides with sites of Br-UTP incorporation (Fig. 3, top row). In fact, the Br-UTP incorporation is often more prominent in the PNC than in most of the nucleoplasm. However, the size and shape of the sites of Br-UTP incorporation often do not completely overlap with the PNC. The incorporation was inhibited when it was performed at 4°C and was not detected in the presence of RNase A (data not shown), suggesting that the nucleotides are incorporated into the RNA in an energy-dependent reaction. The nucleotide incorporation could result from either transcription or posttranscriptional modification of nascent RNA, including editing and uridinylation. It has previously been shown that U is posttranscriptionally added to certain small RNA polymerase III transcripts, including RNase MRP RNA (Hashimoto and Steitz, 1983; Yuan et al., 1989), which is found in the PNC. To determine the nature of the Br-UTP incorporation in the PNC, we examined whether the incorporation is DNA dependent and whether the PNC incorporates nucleotides other than Br-UTP. We found that the Br-UTP incorporation in the PNC and the entire nucleus (Fig. 3, second row) was inhibited in the presence of a high concentration of actinomycin D (50 μg/ml) (Perry, 1963), which intercalates into DNA and prevents it from being used as a transcription template. Furthermore, addition of FITC-CTP to the transcription cocktail resulted in an incorporation in the PNC that is similar to the incorporation of Br-UTP (Fig. 3, third row). These findings further demonstrate that the nucleotide incorporation into the PNC is the consequence of transcription.

To identify which RNA polymerase is involved in the Br-UTP incorporation in the PNC, transcription inhibitors that preferentially inhibit different RNA polymerases were added individually to the transcription cocktail. To inhibit RNA polymerase I activity, two alternative approaches were used. Actinomycin D, which inhibits RNA polymerase I at low concentration (Perry, 1963), was added, and the concentration used was titrated such that the nucleolar incorporation of Br-UTP was significantly reduced and the nucleoplasmic incorporation did not exhibit a detectable change (Fig. 3, fourth row). At this concentration of actinomycin D, no significant change was observed in the Br-UTP incorporation in the PNC (Fig. 3, fourth row). Alternatively, cells were pretreated with cycloheximide (100 μg/ml) for up to 5 h before the Br-UTP incorporation assay. Cycloheximide has been shown to inhibit protein synthesis as well as RNA polymerase I transcription by limiting essential labile factors (Higashi et al., 1968; Willems et al., 1969; O'Keefe et al., 1994). The indirect inhibition of RNA polymerase I by inhibiting protein synthesis enables cycloheximide to circumvent the potential accessibility problem that other drugs might have. The treatment of cycloheximide inhibited most of Br-UTP incorporation in the nucleolus but did not appreciably alter the incorporation in the PNC (Fig. 3, fifth row). The similar results obtained by using two different inhibitory mechanisms suggests that RNA polymerase I is unlikely to be responsible for the Br-UTP incorporation in the PNC. To examine whether RNA polymerases II and/or III are involved, we added α-amanitin into the transcription cocktail. α-Amanitin specifically and selectively inhibits RNA polymerase II at a low concentration of 50 μg/ml (Stripe and Fiume, 1967; Weinmann et al., 1975) and inhibits both polymerases II and III at a high concentration of 300 μg/ ml (Weinmann and Roeder, 1974). Surprisingly, the addition of α-amanitin at either the low or high concentration did not significantly change the Br-UTP incorporation in the PNC (Fig. 3, bottom row), despite a significant reduction in nucleoplasmic incorporation. Since the Br-UTP incorporation in the PNC is due to the transcription that occurs within the 5 min of pulse labeling as described above, and since we have ruled out the involvement of RNA polymerase I transcription, it is therefore most likely that RNA polymerase II and/or III are responsible for the synthesis of nascent RNA in the PNC. A reasonable explanation for a lack of transcription inhibition may be the inability of α-amanitin to gain access into the PNC.

To examine if inhibition of transcription would influence the structure of the PNC in vivo, HeLa cells were treated with α-amanitin at 50 μg/ml for 5 h. The structure of the PNC showed a marked alteration after inhibition of RNA polymerase II (Fig. 4, A and C). The PNC is no longer a compact structure with clear boundaries after α-amanitin treatment. PTB (green) seems to extend from what appears to be the original site of the PNC into the nucleoplasm and, in many cases, forms a series of dots in a rosette with a hollow center (Fig. 4,A, arrow and arrowhead; area at the arrow is enlarged in the inset). When double labeled with the anti-Sm antibody (red), a colocalization was observed between the original sites of the PNC and snRNPs. Interestingly, the extended rosette-shaped dots surround the round snRNP clusters (Fig. 4,C, arrow and arrowhead; area at the arrow is enlarged in the inset). Such alterations appear to form a gradient that decreases with distance from the original locus (the strongly stained region) of the PNC. In contrast, inhibition of RNA polymerase II transcription exerts little to no effect on the diffuse nuclear distribution pattern of PTB in cells that do not have a PNC (Fig. 4 D), demonstrating that the observed alteration is specific to the PNC. Similar changes were also observed when cells were treated with DRB, another RNA polymerase II inhibitor that inhibits a major nuclear Ser/Thr protein kinase, casein kinase II (Sehgal et al., 1976; Zandomeni and Weinmann, 1984). These changes were reversible after cells were grown in drug-free medium for 2 h (data not shown), indicating that the observed alteration in the structure of the PNC is unlikely to be the result of cell death. These findings show that the integrity of the PNC is dependent upon the transcriptional activity of RNA polymerase II.

Examination of another hnRNP protein, CUG-BP/ hNab50, during transcription inhibition using monoclonal antibody 3B1 (Timchenko et al., 1996), which specifically recognizes CUG-BP/hNab50, revealed a similar reorganization of the PNC. However, in contrast to PTB, most of the soluble nucleoplasmic CUG-BP/hNab50 is localized to the cytoplasm when RNA polymerase II transcription is inhibited by α-amanitin. This finding suggests that CUG-BP/hNab50 may belong to the group of hnRNPs that shuttle between the nucleus and cytoplasm in a transcription-dependent manner (for review see Siomi and Dreyfuss, 1997). However, the fraction of CUG-BP/hNab50 that is present in the PNC remains in the nucleus and is colocalized with PTB in the structurally altered PNC (Fig. 4, G–I). In cells that do not contain a PNC, CUG-BP/hNab50 is not detected in the nucleus upon transcription inhibition (data not shown).

When cells in culture were treated for 2–5 h with actinomycin D at a concentration that either selectively inhibits RNA polymerase I (0.04 μg/ml) or all RNA polymerases (10 μg/ml) (Perry, 1963), the PNC was no longer detected by immunolabeling using monoclonal antibodies SH54 or 3B1 (data not shown). However, when cells were treated with cycloheximide (a protein synthesis inhibitor) at 100 μg/ml for up to 5 h, little change was observed in the structure of the PNC (data not shown). Since cycloheximide also inhibits RNA polymerase I activity by inhibiting the synthesis of necessary labile factors (Higashi et al., 1968; Willems et al., 1969; O'Keefe et al., 1994), the resistance to cycloheximide treatment suggests that the structural integrity of the PNC is not dependent on RNA polymerase I transcription or protein synthesis. This finding is consistent with the observation in permeabilized cells that the Br-UTP incorporation in the PNC does not reflect RNA polymerase I transcription. As previous studies showed that treatment with actinomycin D causes nucleolar fragmentation (Reynolds et al., 1964; Ochs et al., 1985), it is not clear whether the disappearance of the PNC after actinomycin D treatment is due to other effects of the drug rather than the inhibition of RNA polymerase I activity.

Incorporation of Br-UTP together with the presence of RNA transcripts and hnRNP proteins in the PNC suggest that the PNC is involved in RNA metabolism. To further investigate the function of the PNC, we examined it for the presence of polyadenylated RNA, pre-mRNA splicing factors, and a 3′ end processing factor. In situ hybridization in HeLa cells using a biotinylated oligo (dT)₅₀ probe (Huang et al., 1994) revealed that poly(A) RNA is present in the PNC in addition to being distributed throughout the nucleus in a diffuse and speckled pattern (Fig. 5, top row). The labeling of the poly(A) RNA in some PNCs is at a similar intensity as the larger nuclear speckles. In other PNCs, the labeling intensity of poly(A) RNA is indistinguishable from the diffuse nuclear labeling (data not shown).

Immunolabeling of pre-mRNA splicing factors including U2 snRNPs (Habets et al., 1987, 1989), SC35 (Fu and Maniatis, 1990), and a 3′ end processing factor, PAB II (Krause et al., 1994), showed that these factors are present in the PNC in addition to their previously characterized sites of localization (Fig. 5). However, the labeling intensity varies among PNCs. To exclude the possibility that the labeling in the PNC is simply due to the diffuse nuclear staining of these factors, we examined the localization of another diffusely distributed nuclear component, p80 coilin. Coilin, an 80-kD protein, is diffusely distributed in the nucleus in addition to being present in coiled bodies (for reviews see Brasch and Ochs, 1992; Lamond and Carmo-Fonseca, 1993; Gall et al., 1995; Roth, 1995). When coilin was localized with anticoilin antibody (Andrade et al., 1993), no staining of PNCs was observed (Fig. 5, bottom row). The presence of RNA processing factors and poly(A) RNA in the PNC is consistent with the idea that the PNC is a site of transcription and that RNA polymerase II is one of the transcription systems involved. Furthermore, these findings suggest that posttranscriptional processing of certain transcripts may also occur in the PNC.

To understand the dynamics of the hnRNP proteins in the PNC, we used FRAP to examine the turnover of GFP– PTB in the PNC (see Materials and Methods). Cells transfected with the GFP–PTB construct were examined using a confocal laser-scanning microscope (Carl Zeiss, Inc., Thornwood, NY). Cells with two PNCs were chosen so that one of them served as a marker to monitor the specificity of bleaching and the stability of the focal plane. An initial image was captured before photobleaching. The PNC was photobleached for 20 s by exposure to the 488-nm laser line using the line scanning mode. An averaged image was obtained immediately after photobleaching followed by a series of images at different time points (Fig. 6, top and middle rows). The photobleaching resulted in a nearly complete loss of the GFP–PTB labeling in the targeted PNC. The bleaching was specific since the neighboring PNC, which was separated by a few micrometers, was not affected. 25 s after the bleaching, the GFP–PTB began to reappear in the PNC, and the fluorescent intensity in the PNC recovered to a similar level as before the bleaching process within 5 min. The rapid recovery suggests that the unbleached GFP–PTB in the nucleoplasm quickly enters the PNC. Moreover, the quantitatively large degree of recovery indicates that GFP–PTB is highly mobile in the PNC and that there is not a large immobile fraction of the protein. To exclude the possibility that the recovery of the GFP–PTB labeling in the PNC is due to a spontaneous fluorescence recovery of GFP–PTB, fixed cells expressing GFP–PTB were examined by FRAP in an identical manner (Fig. 6, bottom row). Again, a complete photobleaching of the labeled PNC was achieved without affecting an adjacent PNC. However, recovery of the fluorescence in the bleached PNC was not observed up to 30 min. The result of the control experiment confirmed that the fluorescence recovery observed in living cells is most likely due to the rapid turnover of PTB in the PNC. The rapid turnover of this hnRNP protein in the PNC is consistent with the dynamic nature of a transcription site with regard to RNA synthesis and subsequent transport of processed product away from the transcription site.

To determine the solubility of the PNC, HeLa cells were first extracted with 0.5% Triton X-100, followed by treatment with 250 mM ammonium sulfate and subsequent DNase I digestion (Fey et al., 1986). Cells were then fixed and immunostained with SH54, a previously characterized monoclonal antibody that specifically recognizes PTB in the PNC (Huang et al., 1997), and human antifibrillarin antibody (Sigma Chemical Co.) (Ochs et al., 1985), which marks the nucleolus. PTB in the PNC remains detectable at the periphery of the nucleolus after the extraction procedure (Fig. 7,A, arrowhead). The PNCs in these preparations appear to be more rounded and smaller in size than in unextracted cells. In contrast to the pool of PTB in the PNC, the diffusely localized nucleoplasmic pool of PTB decreased significantly upon extraction, concomitant with an increase in the staining of the protein in the nucleolus (Fig. 7,A), which was identified by immunolabeling with the antifibrillarin antibody (Fig. 7,B). To examine whether PTB in the nucleolus is derived from the PNC, Detroit 551 cells (normal human fibroblasts), only 2% of which display visible PNCs, were prepared using the same protocol. A similar relocation of nucleoplasmic PTB to the nucleolus was observed in all of the cells in spite of the absence of the PNC in these cells (Fig. 7 D). The simplest explanation is that the extraction leads to the release of PTB from binding to components that are responsible for its diffuse nuclear distribution pattern, and it is then relocated into the nucleoli. These observations demonstrate that the PNC-associated PTB represents a less soluble fraction than the diffuse nuclear population of this protein.

In the present study, we have shown that the PNC actively incorporates Br-UTP and FITC-CTP in a transcription assay using permeabilized cells. Many studies have used this assay to investigate transcription patterns in the cell nucleus (Hozak et al., 1994; Aoki et al., 1997; Fay et al., 1997; Neugebauer and Roth, 1997) since its initial establishment (Jackson et al., 1993; Wansink et al., 1993). Our observation that the PNC actively incorporates labeled nucleotides in a DNA-dependent manner after 5 min of pulse labeling suggests that the PNC is a site of transcription. Inhibition of RNA polymerase I either by addition of actinomycin D in the transcription cocktail or by pretreatment of cells with cycloheximide does not affect the Br-UTP incorporation, indicating that transcription of nascent RNA in the PNC is unlikely to involve RNA polymerase I. This finding is consistent with the report by Matera et al. (1995) that 28S rRNA was not detected in the PNC using in situ hybridization and our previous findings that fibrillarin, which is required for rRNA processing, is not present in the PNC (Huang et al., 1997). RNA polymerases II and/or III may be responsible for the transcription occurring in the PNC, although it is not clear at the present time whether both polymerases are involved. Consistent with this suggestion are the findings that poly(A) RNA and small RNAs transcribed by RNA polymerase III, including hY RNAs, RNase MRP RNA, and RNase P RNA (Matera et al., 1995), are detected in the PNC. Furthermore, immunocytochemical labeling revealed that RNA processing factors, including snRNPs, SC35, and PAB II, are present in the PNC. SnRNPs and SC35 primarily participate in the processing of RNA polymerase II transcripts, and PAB II binds to polyadenylated RNA transcribed by both RNA polymerase II and III. It has become increasingly evident from morphological and biochemical studies that RNA transcription and processing are spatially and temporally linked (Beyer et al., 1980; Beyer and Osheim, 1988; Jiménez-García and Spector, 1993; Xing and Lawrence, 1993; Zhang et al., 1994; Bauren et al., 1996; Huang and Spector, 1996; Du and Warren, 1997; Kim et al., 1997; McCracken et al., 1997; Misteli et al., 1997; Zeng et al., 1997). The presence of RNA processing factors in the PNC supports the notion that the PNC is a site of transcription and suggests that it may also be involved in RNA processing. However, we cannot exclude the possibility that the rapid accumulation of newly synthesized RNA transcripts in the PNC may be the result of transcription elsewhere in the nucleus and the subsequent very rapid translocation of these transcripts to the PNC. As described in a previous study by Matera et al. (1995), the chromosome segment that encodes two of the hY RNAs only showed an occasional association with the PNC. In addition, the La protein known to be at least transiently associated with newly synthesized RNA polymerase III transcripts was not detected in the PNC using immunocytochemical labeling (Matera et al., 1995). Very recently, two other nuclear bodies were found to incorporate tagged nucleotides after a short pulse labeling (LaMorte et al., 1998; Pombo et al., 1998). Promyelocytic leukemia (PML) bodies and coiled bodies rapidly accumulate FITC-UTP upon microinjection into cells, and PML bodies were also shown to contain a transcription factor, cAMP-regulated enhancer binding protein (CREB) binding protein (LaMorte et al., 1998). In addition, the polymorphic interphase karyosomal association (PIKA) domain was shown to be associated with specific chromosomes and to also be active in transcription (Pombo et al., 1998). These observations, together with our finding that the PNC accumulates nascent RNA, suggest that transcription may be spatially regulated in subnuclear compartments. Further studies will identify transcripts that are synthesized and/or processed in the PNC.

Based upon the extraction behavior and structural alterations during transcription inhibition, two populations of the hnRNP proteins PTB and CUG-BP/hNab50 were identified in the HeLa cell nucleus. One population is diffusely distributed throughout the nucleoplasm, and the other population is enriched in the PNC with a much higher fluorescent intensity, implying a higher protein concentration. The PNC-associated hnRNP proteins are linked with the less soluble fraction of the nucleus and remain associated with the structurally altered PNC during transcription inhibition, whereas the diffusely distributed nuclear populations are removed by the extraction, and CUG-BP/hNab50 is relocated to the cytoplasm during transcription inhibition. These differences suggest that the two populations of hnRNP proteins, the PNC-associated and the diffuse nucleoplasmic, each may interact with a different set of cellular constituents. Since the PNC is predominantly observed in cells with a transformed phenotype, we speculate that the PNC-associated hnRNP proteins may be complexed with cellular components that are altered in terms of their expression or modification in transformed cells. Future studies will focus on the isolation and identification of these constituents.

An increasing number of nuclear bodies or inclusions have been described in recent years from cells or tissues that have altered physiology or are derived from various disease-related samples. For example, coiled bodies, round and electron-dense structures, are often observed in transformed and cancer cell lines (Spector et al., 1992; Ochs et al., 1994). Coiled bodies contain snRNPs, U3 snoRNP, fibrillarin, NOPP140, and p80-coilin (for reviews see Lamond and Carmo-Fonseca, 1993; Gall et al., 1995; Roth, 1995). Several snRNA genes (U1, U2, and U3) are localized adjacent to coiled bodies in a percentage of cases (Frey and Matera, 1995; Smith et al., 1995; Gao et al., 1997). Recently, LaMorte et al. (1998) have localized nascent RNA in coiled bodies, and a transcription factor, TFIIH, was also detected in coiled bodies (Jordan and Carmo-Fonseca, 1997). However, the exact function of coiled bodies remains unknown. A second nuclear structure, “gems” (gemini of coiled body), was shown to be frequently associated with coiled bodies (Liu and Dreyfuss, 1996). Gems contain the survival of motor neurons (SMN) protein that is encoded by a gene responsible for spinal muscular atrophy (Liu et al., 1997). The SMN protein was shown to interact with snRNPs that are involved in pre-mRNA splicing and with a cellular protein called SIP1 through a separate interaction (Liu et al., 1997). The SMN–SIP1 complex was shown to be involved in snRNP biogenesis (Fischer et al., 1997; Liu et al., 1997). PML bodies, also named ND10 (nuclear domain 10) and POD (PML oncogenic domains), change their number and size in acute promyleocytic leukemia (Ascoli and Maul, 1991; Dyck et al., 1994; Koken et al., 1994, 1995; Weis et al., 1994; Terris et al., 1995; for review see Doucas and Evans, 1996). Generally, each cell nucleus contains ∼10–20 PML bodies ranging from 0.3 to 1 μm in diameter. In acute promyleocytic leukemia cells, PML bodies break up into a large number of microparticulates (Dyck et al., 1994). Recently, LaMorte et al. (1998) have localized nascent RNA polymerase II transcripts and CREB binding protein to a subset of PML bodies, suggesting that at least some PML bodies are involved in transcription. Nuclear inclusions, containing Huntington protein, are found in neurons involved in Huntington's Disease (Davies et al., 1997). Patients with Huntington's Disease have an expanded NH₂-terminal polyglutamine region in Huntington, and its length influences the extent of Huntington accumulation within the intranuclear inclusions (DiFiglia et al., 1997). The presence of ubiquitin in these structures suggests that the abnormal Huntington is targeted for proteolysis (DiFiglia et al., 1997). Another recent example of a disease-related nuclear inclusion is the change in the subnuclear localization of the ataxin-1 protein, which is associated with the neurodegenerative disorder, Spinocerebellar ataxia type I. The disease-related mutant ataxin-1, with an expanded polyglutamine tract, localizes to a single ∼2-μm structure compared with the normal ataxin-1 protein, which localizes to several 0.5-μm nuclear structures (Skinner et al., 1997). Ataxin-1 interacts with a cerebellar leucine-rich acidic nuclear protein in a manner such that the affinity of the association depends upon the number of glutamines in mutant ataxin-1 (Matilla et al., 1997). All of these examples demonstrate that nuclear structure is altered in response to changes in cellular physiology and/or pathology of cells or tissues. These changes may reflect changes of nuclear function and/or regulation. Although many nuclear bodies and inclusions have been described morphologically, the functional relationship between many of these structural changes and the respective diseases that they are associated with are not clear. Our finding that the PNC is potentially involved in transcription gives us an important clue to further address the molecular basis of the PNC and its relationship with the transformed phenotype.

We would like to thank Tamara Howard for her enthusiastic technical assistance. We are very grateful to Dr. Maurice S. Swanson for the 3B1 antibody.

DRB

5,6-dichloro-1-β-d-ribofuranosylbenzimidazole

FRAP

fluorescence recovery after photobleaching

GFP

green fluorescent protein

hnRNP

heterogeneous ribonucleoprotein

PAB II

poly(A) binding protein II

PML

promyleocytic leukemia

PNC

perinucleolar compartment

PTB

polypyrimidine binding protein

SMN

survival of motor neurons