Nuclear Pore Complex Is Able to Transport Macromolecules with Diameters of ∼39 nm (original) (raw)

Abstract

Bidirectional transport of macromolecules between the nucleus and the cytoplasm occurs through the nuclear pore complexes (NPCs) by a signal-mediated mechanism that is directed by targeting signals (NLSs) residing on the transported molecules or “cargoes.” Nuclear transport starts after interaction of the targeting signal with soluble cellular receptors. After the formation of the cargo-receptor complex in the cytosol, this complex crosses the NPC. Herein, we use gold particles of various sizes coated with cargo-receptor complexes to determine precisely how large macromolecules crossing the NPC by the signal-mediated transport mechanism could be. We found that cargo-receptor-gold complexes with diameter close to 39 nm could be translocated by the NPC. This implies that macromolecules much larger than the assumed functional NPC diameter of 26 nm can be transported into the karyoplasm. The physiological relevance of this finding was supported by the observation that intact nucleocapsids of human hepatitis B virus with diameters of 32 and 36 nm are able to cross the nuclear pore without disassembly.

INTRODUCTION

Bidirectional transport of macromolecules between the nucleus and the cytoplasm is a major and essential activity in eucaryotic cells. The double nuclear membrane, which separates the nucleoplasm from the rest of the cell, contains specialized channels called nuclear pore complexes (NPCs) through which nuclear import and export occur (reviewed by Mattaj and Englmeier, 1998; Nakielny and Dreyfuss, 1999; Wente 2000). NPCs allow passive diffusion of ions and small molecules through aqueous channels with a diameter of ∼9 nm (Paine et al., 1975). Molecules larger than this diffusion limit are selectively transported in and out of the nucleus by a signal-mediated process (De Robertis et al., 1978; Dingwall et al., 1982). Signals mediating import of nuclear proteins (called nuclear localization sequences or NLSs) were identified more than two decades ago (Dingwall et al., 1982). Early studies in cells injected with various sizes of gold particles coated with the NLS-bearing protein nucleoplasmin showed that the NPC can import NLS-coated gold particles that are up to ∼26 nm in diameter (including the protein coat; Dworetzky et al., 1988), which resulted in the general belief that this diameter reflects the threshold size for karyophilic macromolecules crossing the NPC. More recently, it has been shown that the NLSs on the macromolecule or “cargo” to be transported are recognized by soluble receptor proteins, and that the cargo-receptor complex crosses the NPC (Görlich et al., 1994, 1995; Moroianu et al., 1995; Radu et al., 1995). Therefore, it is expected that after cytoplasmic injection of NLS-coated gold particles into cells, the NLS-coated gold particles will be modified by the binding of intracellular import receptors to the NLSs. Consistent with this, the interaction between the two receptors, termed importin (karyopherin) α and β, for classical NLSs, was speculated to increase the diameter of the transported complex by ∼8 nm (Ribbeck and Görlich, 2001).

The knowledge of the exact functional diameter of the NPC is very important in the field of virology. Many viruses that infect eucaryotic cells replicate in the nucleus. During infection, these viruses have to cross the NPC. This is achieved by mimicking cellular NLSs and by using the cellular import receptors to cross the NPC (reviewed by Kasamatsu and Nakanishi, 1998; Whittaker and Helenius, 1998; Whittaker et al., 2000). However, based on the previous reported value for the functional diameter of the NPC (Dworetzky et al., 1988), it has been assumed that viruses >26 nm have to disassemble into small components before they cross the NPC. For example, because the genome-containing nucleocapsids of hepatitis B viruses (HBVs) (also termed cores), which replicate their viral DNA inside the nucleus of the infected cell, have diameters of 32 or 36 nm (dependent upon their symmetry; Crowther et al., 1994; Kenney et al., 1995), it has been assumed that they are too big to cross the NPC without disassembly. Thus, the current hypothesis by which HBV delivers its genome into the cell nucleus is that the core particles disassemble at the cytoplasmic face of the NPCs where a complex of viral DNA and covalently bound polymerase is released, followed by the nuclear import of the genome, mediated by the viral polymerase (Kann et al., 1997). These assumptions are thought to be true not only for the initial infection of the cell but also for the delivery of progeny genomes from the cytosol into the already infected nucleus, which amplifies nuclear viral DNA leading to persistent infection on the cellular level. Consistent with this model, it has been shown by indirect immunofluorescence microscopy that _Escherichia coli_-grown HBV cores bind to the NPCs of digitonin-permeabilized cells without migration into the free karyoplasm (Kann et al., 1999). These recombinant HBV core particles, used by Kann et al. (1999), are morphologically and immunologically identical to authentic virus-derived core particles (Kenney et al., 1995). However, in contrast to authentic cores, they do not contain either the viral DNA or the polymerase, but bacterial RNA. Kann et al. (1999) have also shown that the _E. coli_-expressed HBV core particles only bind to the NPC of permeabilized cells when they are phosphorylated, and that NPC binding is also mediated by importin α and β. Because these studies by indirect immunofluorescence microscopy lack the resolution necessary to visualize the docking of the HBV cores to single nuclear pores, electron microscopy (EM) studies of the NPC docking of HBV cores are necessary to identify where at the NPC the core particle disassemble and what is the strategy followed by HBV to release its genome into the cell nucleus.

In the present study we have structurally characterized cargo-receptor–coated gold particles and used them in import assays to directly determine the functional diameter of the NPC. We found that cargo-receptor–gold complexes as large as 39 nm in diameter (including the cargo-receptor coat) can be imported into the nucleus by the NLS-mediated transport mechanism. To show the physiological relevance of our findings we then studied nuclear import of human HBV nucleocapsids. Consistent with our results with cargo-receptor–gold complexes we found that intact HBV capsids with diameters of 32 and 36 nm are able to cross the NPC without disassembly.

MATERIALS AND METHODS

Gold Particles and Protein-Gold Complexes

Colloidal gold particles with diameter of 22 ± 2, 26 ± 3, and 36 ± 4 nm were prepared by reduction of tetrachloroauric acid with sodium citrate (Frens, 1973). Nucleoplasmin (NP) was kindly provided by Dr. Dirk Görlich, Zentrum für Molekulare Biologie der Universität Heidelberg, University of Heidelberg, Germany.

Gold particles were coated with NP or bovine serum albumin (BSA; Sigma, St. Louis, MO) according to Baschong and Wrigley (1990) with some modifications. Namely, protein was added to the colloidal gold solution, while stirring, to an amount that exceeded 10 times the minimal stabilization amount to ensure that the gold particles were fully stabilized and would not increase their coat size by attracting nonspecific proteins upon injection into cells. The protein-gold complexes were then centrifuged at 45,000 × g for 15 min, and the soft pellet was resuspended in low-salt buffer (LSB; 1 mM KCl, 0.5 mM MgCl2, 10 mM HEPES, pH 7.5) and used immediately for microinjection.

To form the NP-receptor–gold complex, both NP- and BSA-coated gold particles were incubated at 4°C for 2 h with an excess of importin α. The gold complexes were centrifuged at 45,000 × g for 15 min and the soft pellet was resuspended in LSB. The importin α-incubated gold complexes were further incubated at 4°C for 2 h with an excess of importin β. The resulting gold complexes were centrifuged at 45,000 × g for 15 min, and the soft pellet was resuspended in LSB and used immediately for microinjection.

Negative Staining

To measure the size of the protein coat of the gold-protein complexes, these were negatively stained and examined in the electron microscope. For this purpose, the gold-protein complexes were adsorbed for 2 min onto glow-discharged carbon-coated pallodion films on copper EM grids. The grids were then washed on 3 drops of LSB before they were negatively stained with 0.75% uranyl formate for 1 min.

Immunogold Labeling

For immunogold labeling, colloidal gold particles, ∼8 nm in diameter, were prepared as described (Slot and Geuze, 1985), and an anti-importin β antibody was conjugated to the colloidal gold particles as described (Baschong and Wrigley, 1990). The importin α- and β-incubated gold particles were adsorbed for 2 min onto glow-discharged carbon-coated pallodion films on copper electron microscopy grids, and the grids were incubated with the gold-coupled antibody for 1 h at room temperature. After incubation, the grids were washed on three drops of LSB and were negatively stained with 0.75% uranyl formate for 1 min.

HBV Core Particles

HBV core particles were obtained from G. Borisova and P. Pumpens (Biomedical Research and Study Center, Riga, Latvia) and phosphorylated according to Kann and Gerlich (1994).

Electron Microscopy Import Assay in Xenopus laevis Oocytes

Mature (stage 6) oocytes were surgically removed from X. laevis as described previously (Panté_et al._, 1997). Fresh-made gold-protein complexes (∼50 nl) or HVB core particles were microinjected into the cytoplasm of the oocytes. Injected oocytes were then incubated at room temperature in modified Barth's saline buffer [88 mM NaCl, 1 mM KCl, 0.82 mM MgSO4, 0.33 mM Ca(NO3)2, 0.41 mM CaCl2, 10 mM HEPES, pH 7.5] for 1 h (NP-injected oocytes) or 15–30 min (HVB-injected oocytes). The oocytes were prepared for embedding in Epon 812 resin (Fluka, Buchs, Switzerland) as described by Panté_et al._ (1997). Ultrathin sections were collected on pallodion/carbon-coated copper EM grids and were stained by conventional procedures (Panté_et al._, 1997).

Electron Microscopy and Quantitation

All micrographs were digitally recorded in a Hitachi H-7000 transmission electron microscope (Hitachi, Tokyo, Japan) operated at an acceleration voltage of 100 kV. Magnification calibration was performed as described (Wrigley, 1968).

The sizes of the gold particles and their protein coats were determined from digital electron micrographs of negative stained preparations by using Adobe Photoshop 5.5 (Adobe Systems, Mountain View, CA). The diameter of gold particles in the nucleus of injected Xenopus oocytes and HBV core particles was determined from digital electron micrographs revealing cross sections of NPCs along the nuclear envelope.

RESULTS

Cargo-Receptor Coat Can Add an Additional 13 nm to Diameter of Gold Particles

To determine precisely how large macromolecules crossing the NPC by the signal-mediated transport mechanism could be, we coated gold particles of various sizes with import cargoes and their import receptors and determined the exact size of the cargo-receptor coat by high-resolution electron microscopy. For these experiments we used nucleoplasmin (a nuclear protein from X. laevis oocytes containing two classical NLSs of basic amino acids), and the receptor for classical NLS, which consists of two functionally different subunits (importin [karyopherin] α and β). As illustrated in Figure 1 (also Table 1), for gold particles of 22–36 nm in diameter, the protein coating contributed to a low-density layer that surrounds the gold particles, which was revealed by contrasting the protein-gold complexes with uranyl formate (i.e., by negative staining). Whereas the thickness of this layer was only ∼4 nm on each side (Table 1) when the protein coat consisted of BSA, this layer was 6.6 nm in average (5.2–8.3 nm/side) for NP, reflecting the different molecular mass of BSA (68 kDa) and NP (165 kDa). The observed protein layers are in the same order of the protein layer of cocanavalin A (108 kDa), which is a 4- × 8-nm molecule and yielded gold particles with a 4-nm coat (Horisberger and Rosset, 1977). However, it must be considered that the interactions of proteins and colloidal gold depend not only on the molecular mass of the protein but also on a combination of many factors, including shape, electrical charge, and hydrophobic properties of the protein.

Figure 1.

Electron microscopy of representative gold particles and their protein coat. Gold particles (A, 22 nm; B, 26 nm; and C, 36 nm) uncoated (first row) and coated with NP or BSA (second row) were visualized in the electron microscope by negative staining. The third and fourth rows are examples of NP- and BSA-coated gold particles that were incubated first with importin α (NP + α and BSA + α) and then with importin β (NP + α + β and BSA + α + β). The last row shows examples of NP- and BSA-coated gold particles that were incubated with importin α and β and then immunogold labeled with an anti-importin β antibody directly conjugated with 8-nm gold particles.

Table 1.

Thickness of the protein coat (nm) surrounding the gold particles

As we expected, when these NP-coated gold particles were incubated in vitro with importin α, the association of importin α to the NLSs of NP-coated gold particles increased the protein layer around the gold particles by 1.3–3 nm (on average) per radius (Figure 1, row 3; and Table 1). In contrast, the protein coat of the gold particles remained more or less constant for BSA-coated gold particles that were incubated in vitro with importin α (Figure 1 and Table 1).

The NP-importin α layer that surrounded the gold particles was less compact than the NP layer, and varied in thickness even on the same gold particle (which is reflected in the large values for the SD). This variability was expected in agreement with the random adsorption of NP onto the surface of the gold particles. In addition, the size of the NP-importin α was predicted from the geometry of importin α and the way it accommodates the NLSs of NP. Importin α is an elongated molecule with a cylindrical shape of 10 × 3 nm and can accommodate the bipartite NLS of NP within the center of the molecule (Conti et al., 1998). The two NLS-binding sites are located at ∼2 and 3 nm from each end of the molecule. Thus, if the binding of importin α to the NP-coated gold particles is in a “side-on” orientation, <2 nm (i.e., the radius of the cylindrical molecule) will be added to the NP-layer per side. On the other hand, if importin α is added in an end-on orientation most of the importin α molecule will be embedded on the NP coat and only 2 or 3 nm from the importin α molecule will be added to the previous NP coat.

As illustrated (Figure 1, row 4; Table 1), when these gold-NP–importin α complexes were incubated in vitro with importin β, the binding of importin β to importin α on these gold particles contributed an additional 0.3–0.6 nm in average to the protein layer per radius. This low increment in the protein coat was expected because when importin β interacts with the importin β-binding domain of importin α, it is embedded within the structure of importin β (Cingolani et al., 1999). Again, there was no increase in the thickness of the protein layer in the control experiments with BSA-coated gold particles that were incubated in vitro first with importin α and then with importin β. Similar to the gold-NP–importin α complex, the gold-NP–importin α-β complex has a very heterogeneous protein coat (Figure 1, row 4), which is a consequence of the irregular coat from the gold-NP-importin α particles. Taken together, these results indicate that the incorporation of importin α and β into NP-coated gold particles increased the protein coat by 1.9–3.3 nm/radius on average. However, in some cases the total NP-importin α and β layer was as large as 13.6 nm (Table 1).

To obtain further evidence of the extra layer contributed by the two subunits of the import receptor, we used an anti-importin β antibody conjugated with 8-nm-diameter gold particles to locate importin β within the gold-NP–receptor complex. As shown in Figure 1, this antibody labeled the NP-coated gold particles that were incubated with importin α and importin β, but not BSA-coated gold particles that were also incubated with importin α and importin β. For the gold-NP-α-β complex, the distance between the large gold particle (coated with NP) and the 8-nm antibody-coupled gold particle was 8–10 nm. These values agree with the thickness of the cargo-receptor layer that surrounds the gold particles as measured after negative staining (Figure 1 and Table 1).

Nuclear Import of Large NP-coated Gold Particles

Our results of the thickness of the protein coat surrounding NP-receptor–coated gold particles clearly document that the binding of importin α and importin β to the NP-coated gold particles increase the diameter of the protein-gold complexes. Because the protein coat surrounding the gold particle cannot be resolved in electron micrographs of plastic-embedded and sectioned cells, it is very important to know precisely the exact size of the protein coat that surrounds the gold particle before they are injected into cells. To accurately determine the functional diameter of the NPC, we microinjected our NP-gold particles (of known protein coat; Figure 1) into the cytoplasm of Xenopus oocytes, and followed their fate by electron microscopy. As demonstrated previously (Feldherr et al., 1984; Richardson et al., 1988; Panté_et al._, 1996), NP-coated gold particles were targeted to the NPCs and, depending on the size of the gold particles, were imported into the nucleus (Figure 2). In contrast, BSA-coated gold particles remained in the cytoplasm. We found that 1 h after injection, 36% of NP-gold particles with diameter of 22 ± 2 nm (without the NP coat) were imported into the nuclei of Xenopus oocytes (Figures 2A and 3A and Table 2). Similarly, 28% of NP-gold particles with diameter of 26 ± 3 nm reached the Xenopus nuclei (Figures 2B and 3B and Table 2). In contrast, NP-gold particles with diameter of 36 ± 4 nm were excluded from the nucleus of Xenopus oocytes. However, these last particles were able to associate with the cytoplasmic face of the NPC (Figure 2C). The difference in the efficiency of nuclear import for gold particles of 22 ± 2 and 26 ± 3 nm in diameter is consistent with the notion that large particles diffuse more slowly through the cytoplasm than small particles. Thereby, at any given time after injection more gold particles reached the NPCs in oocytes injected with 22-nm NP-gold than in those injected with 26-nm NP-gold particles.

Figure 2.

Nuclear import of NP-coated gold particles into Xenopus oocyte nuclei. Gold particles of 22 ± 2 nm (A), 26 ± 3 nm (B), and 36 ± 4 nm (C) in diameter were coated with NP and their nuclear import was followed by electron microscopy 1 h after injection into the cytoplasm of Xenopus oocytes. Shown are views of nuclear envelope cross sections with adjacent cytoplasm (c) and nucleoplasm (n). Arrowheads point to gold particles that reached the nucleus or are associated with the nuclear face of the NPC. Gold particles 28 nm in diameter or smaller (without the protein coat) were imported into the nucleus. Bar, 100 nm.

Figure 3.

Histograms on the size distribution of gold particles available for import (total), and found within the cytoplasm and the nucleus. Twenty-two ± 2 nm-gold particles, coated with NP (A), 26 ± 3 nm-gold particles, coated with NP (B), 22 ± 2 nm-gold particles, coated with NP and importin α and β (C), and 26 ± 3 nm-gold particles, coated with NP and importin α and β (D). For comparison, only 100 particles in the nucleus and 100 particles in the cytoplasm were measured. The data were derived from microinjections in four different oocytes.

Table 2.

Nuclear import of NP- and NP-receptor-coated gold particles

For gold particles >20 nm in diameter it is very difficult to obtain particles that are homogeneous in size (Slot and Geuze, 1985). This is reflected in the large SD of the diameter of the gold particles used in this study. For example, the 22-nm gold particle preparation contained particles with diameters from 15 to 26 nm; the 26-nm preparation consisted of particles ranging from 19 to 34 nm (Figure 3, A and B). Thus, we could not exclude that only the smaller particles of this gold preparation entered the nucleus.

Therefore, to determine exactly the maximum size of the NP-gold complexes crossing the NPC, we then measured the diameter of those gold particles that reached the nucleus and compared their distribution with those available for nuclear import (i.e., distribution of the particle sizes in the cytoplasm and in the preparations). As shown in Figure 3A, by using the 22-nm NP-gold particle preparation, all gold sizes from 15 to 26 nm were able to enter the nucleus. In accordance, the size distribution was the same for particles in the nucleus, the cytoplasm, and the total available particles (Figure 3A). In contrast, in our NP-gold preparation with an average size of 26 nm, which contained gold particles from 19 to 34 nm, mainly particles 26 nm in diameter or smaller reached the nucleus (Figure 3B) with a low percentage of larger particles, showing a diameter of 28 nm. This resulted in a different size distribution for total, nuclear, and cytoplasmic gold particles and most likely indicated a size limit of the NPC.

To calculate the functional diameter of the NPC, we then considered that these 28-nm NP-gold particles were coated with a protein layer of the minimal size (5.2 nm/radius). Our results indicate that the gated channel, located in the center of the NPC through which macromolecule transport occurs, is able to accommodate NLS-bearing macromolecules as large as 38.4 nm in diameter (28 nm gold + 2 × 5.2-nm protein coat). A more statistical estimation will be taking the size of gold particles that are most frequently found in the nucleus and the average of the NP layer. This will result in a NPC functional diameter that is ∼39 nm (26 nm gold + 2 × 6.6-nm protein coat).

Nuclear Import of NP-Importin α-β-coated Gold Particles

However, it cannot be concluded from the above-mentioned experiments, how many receptor molecules were actually bound by the NP-gold particles during their time within the cytoplasm. The particles might have bound just some molecules, which would not have a significant impact on the size of the complex that passes the nuclear pore, or they might have acquired an entire additional protein shell of importin α and β. Because EM cannot solve the possible variation in the size of the protein coat (see gallery of gold particles in Figure 4B), we incubated our NP-coated gold particles with importin α and importin β (i.e., the gold-NP-α-β complexes, which have a protein coat of 8.5 ± 1.5 nm; Figure 1 and Table 1), and used these in nuclear import assays in Xenopus oocytes.

Figure 4.

Nuclear import of NP-importin α- and β-coated gold particles into Xenopus oocyte nuclei. NP-coated gold particles with diameter of 26 ± 3 nm were incubated in vitro first with importin α and then with importin β. The resulting complexes were injected into the cytoplasm of Xenopus oocytes and their nuclear import was followed by electron microscopy. Shown are low- (A) and high (B)-magnification views of nuclear envelope cross sections with adjacent cytoplasm (c) and nucleoplasm (n). Arrowheads point to gold particles that reached the nucleus or are associated with the nuclear face of the NPC. Gold particles as large as 26 nm in diameter (without the protein coat) were able to cross the nuclear pores and enter the nucleus of Xenopus oocytes. Shown is also a gallery of gold particles that were found in the nucleus of Xenopus oocytes. Bars, 200 nm (A) and 50 nm (B).

Similar to the results with NP-coated gold particles, we found that gold-NP-α-β complexes with gold particles of 22 ± 2, 26 ± 3, and 36 ± 4 nm in diameter were targeted to the cytoplasmic face of the NPC and were imported into the nucleus, depending upon the size. As documented in Table 2, the efficiency of nuclear import of NP-α-β–coated gold particles was comparable with that of NP-gold for both the 22 ± 2- and the 26 ± 3-nm gold preparations.

Similar to the NP-coated gold particles from the 22-nm preparation (Figure 3A), the size distribution of total, nuclear, and cytoplasmic particles was identical for the 22-nm preparation, coated with NP, importin α and β (Figure 3C). Using the 26-nm preparation, in which gold particles of 19–34 nm in diameter were available for import, different distribution between nuclear and cytoplasmic gold was observed (Figure 3D); a difference similar to that obtained for the NP-coated 26-nm preparation (Figure 3B). However, the threshold for the NP-α-β–gold was 26 nm in diameter. Although there were less gold particles with diameter larger than 26 nm in the NP-α-β–gold preparation than in the NP-gold preparation, the divergent threshold for just NP-coated gold particles and the importin α + β + NP-coated gold particles indicates a size difference of ∼2 nm, perfectly reflecting the additional average protein coat of importin α and β of 1.9 nm as shown in Table 1. This divergence supports the concept that after injection of the gold-NP-α–β complex the protein layer does not dissociate before the import through the NPC. However, the diameter of the most frequently imported gold-NP-α-β complexes was 26 nm, as for the just NP-coated particles. This result is in accordance with the high variability of the importin α/β coat, explaining that a large proportion of just NP-coated gold particles have the same size, than gold particles coated with importin α and β additionally.

Nuclear Import of Intact Hepatitis B Virus Cores

To verify the functional diameter of the NPC as well as to show the physiological relevance of this observation we then injected viral capsids in our Xenopus import assay. We chose nucleocapsids (also termed cores) from HBV, a virus capsid that exceeds the size of the previously reported functional diameter of the NPC and therefore were assumed not to cross the NPCs. Similar to the immunofluorescence microscopy studies reported by Kann et al. (1999), we used _E. coli_-expressed core particles that do not disintegrate at the NPC, as shown by using a particle-specific antibody (Kann et al., 1999). For these experiments we first generated phosphorylated recombinant HBV (P-rHBV) cores (unphosphorylated cores do not bind to the NPC; Kann et al., 1999), injected them into the cytoplasm of Xenopus oocytes, and followed their nuclear import by electron microscopy. As we expected, the P-rHBV cores, but not the unphosphorylated rHBV cores, were targeted to and bound by Xenopus NPCs. According to our size determination of the functional diameter of the NPC, but in contrast to the current theory of HBV genome import, we found intact P-rHBV cores lined up inside the central channel of the NPCs and associated with the nuclear side of the NPCs (Figure 5A) but not in the free karyoplasm. The diameter of the P-rHBV cores found in the center of the NPCs and the diameter of those cores that reached the nuclear side of the NPCs were the same as the diameter of the cores found in the cytoplasm or associated with the cytoplasmic face of the NPCs (Figure 5B). The results of these experiments clearly shown that the 32- and 36-nm diameter P-rHBV cores are able to cross the NPC. Thus, and in accordance with previously published data (Kann et al., 1999), these NPC-associated core particles did not disassemble, but remained intact while crossing the NPC.

Figure 5.

Intact hepatitis B virus cores (32 or 36 nm in diameter) are able to cross the nuclear pores. (A) Views of a nuclear envelope cross section with adjacent cytoplasm (c) and nucleoplasm (n) from a Xenopus oocyte that have had phosphorylated recombinant HBV cores microinjected into their cytoplasm. Arrowheads point to core particles associated with the nuclear face of the NPC. (B) Nuclear envelope cross section from a control (noninjected) Xenopus oocyte. (C) Examples of cross-sectioned NPCs with associated HBV cores. (D) Same micrographs as in C but with the nuclear membrane boundaries and the HVB cores outlined. (E) Quantitative analysis of the size of core particles associated with the cytoplasmic face of the nuclear pore (cNPC) or the nuclear face of the nuclear pore (nNPC) from oocytes injected with recombinant HBV cores. 60 HBV cores were measured for each histogram. Bars, 100 nm.

DISCUSSION

In this study we used gold particles coated with cargo-receptor complexes in combination with import assays in Xenopus oocytes and high-resolution electron microscopy to determine the maximum size that macromolecules crossing the NPC by the signal-mediated transport mechanism could be. As the protein coat surrounding the gold particle cannot be resolved in embedding and thin section, we first measured the exact size of the protein coat that surrounds the gold particle before they were used for import assays.

Our results of nuclear import of nucleoplasmin-coated gold particles indicate that using a preparation with particles from 19 to 34 nm in diameter, nearly 50% of the nuclear gold particles showed a size of 26 nm. Due to this high proportion it is most likely that these particles have had a protein coat of the average size, resulting in the cargo size of 39.2 nm (26 + 2 × 6.6 nm). Thus, our best estimation for the functional diameter of the NPC is 39 nm. This value is in accordance with the diameter of the central pore of the NPC, which has been shown to be ∼44 nm in electron microscopy (Hinshaw et al., 1992; Akey and Radermacher, 1993).

These results are in contrast to those of Dworetzky et al. (1988), who have previously shown that the Xenopus oocyte NPC could import gold particles up to ∼23 nm in diameter, coated with a 1.5-nm-measuring shell of nucleoplasmin. However, the striking difference in the size of the protein coat is most likely a consequence of the different protocols used for coating the gold particles with NP. Whereas Dworetzky et al., (1988) used minimal amount of protein to stabilize gold particles, giving a thin protein layer, we used concentration 10 times higher than the minimal stabilization amount, yielding a larger protein layer.

In addition, the use of saturating amounts of protein had the advantage that the gold particles were fully stabilized so that they could not be modified by nonspecific adsorption of cellular proteins or protein complexes of various sizes upon cell injection, resulting in an unpredictable increase of the protein coat. Furthermore, a fully saturated gold surface ensured that particles can only be transported by the soluble import receptors bound to the NLS of NP and not by adsorption of the receptors to the gold particles.

The soluble import receptors importin α and β were first described in 1994 and 1995 (Görlich et al. 1994, 1995; Moroianu et al., 1995; Radu et al., 1995). Thus, the contribution of these receptor proteins that bind to the carrier protein or cargo could not have been considered by Dworetzky in 1988. Therefore, we analyzed the effect of importin α and β on the diameter of cargo-coated gold particles. Our results showed that the protein coat of NP-receptor–coated gold particles is very heterogeneous and has a large variability, resulting in overlapping sizes of just NP and NP-α-β–coated gold. Therefore, it is difficult to define a statistically significant influence of the receptor coat on the diameter of the particles. However, it must be considered that even the contribution of importin α/β to the average diameter of the transported cargo (26-nm gold + 2 × 8.5 protein layer = 43 nm) would be in agreement with electron microscopically determined diameter of the central pore of the NPC (Hinshaw et al., 1992; Akey and Radermacher, 1993).

It could be argued that some other phenomena have occurred that might have interfered with the import of the cargo-receptor-coated gold particles. First, a dissociation of NP from the gold surface might be assumed. However, it is known that protein absorption to gold is irreversible (Leunissen and De May, 1989). In addition, the size distribution of the nuclear gold should not show the sharp size limit as has been observed in our experiments. A second concern might be that importin α and/or β might have dissociated from the NP–gold after microinjection. However, both import receptors are known to show an extremely high affinity. Importin α binds to NP with a _K_D of ∼15 nM and importin β binds to importin α with a _K_D of ∼40 nM (Catimel et al., 2001).

The central pore of the NPC is often, but not always, plugged with a particle of highly variable appearance (called the central plug or transporter). The existence, definite structure, and functional role of such a particle have been discussed (Panté and Aebi, 1993, 1994; Stoffler et al., 1999). However, all our findings suggest that this plug does not play a functional role in restricting the maximal functional diameter of the nuclear pore.

In addition to providing insights in basic cell research, our findings also have a virological impact. The observation that intact HBV capsids are found within the nuclear basket suggests a new model for the transport of the HBV genome into the nucleus, which does not require a disassembly at the cytosolic face of the NPC. Our results supported the idea of Kann et al. (1999) that the P-cores plugged the NPC, preventing the import of other karyophilic substrates. However, it must be considered that these RNA-containing P-cores reflect the immature HBV capsids and not the mature DNA-containing particles. For the latter population a disassembly must be proposed. Whether this disassembly takes place within the nuclear basket or in the free karyoplasm cannot be answered by the present work. In any case, this finding supports the physiological relevance of our data and additionally shows a strategy that may be used by other viruses or capsids for which a disassembly within the cytosol seemed to be a requirement.

Although significant progress has been made in identification and molecular characterization of the receptor for the classical NLS pathway (as well as their crystalline structures, which have recently been resolved; reviewed by Chook et al., 1999; Conti and Izaurralde, 2001), very little is known about the precise molecular mechanism for nuclear import of NLS-bearing proteins through the NPC. The knowledge that the NPC is able to transport macromolecules that are close to 40 nm in diameter, instead of 26 nm in diameter, might be a helpful fact for the evaluation of molecular models proposed for translocation through the nuclear pore.

ACKNOWLEDGMENTS

We are most grateful to Ari Helenius for generous support, for making many constructive suggestions, and for critical reading of the manuscript. We thank Dirk Görlich for providing nucleoplasmin, importin α and β, and the anti-importin β antibody; and Paul Pumpens and Gallina Borisova (Biomedical Research and Study Center, University of Latvia, Riga, Latvia) for providing the purified _E. coli_-derived core particles. This work was supported by a grant of the Deutsche Forschungsgemeinschaft to M.K. (SFB 535, B5), a grant from the Swiss National Science Foundation to N.P. (3100-053034), and a grant from the Natural Sciences and Engineering Research Council of Canada to N.P.

Abbreviations used:

BSA

bovine serum albumin

EM

electron microscopy

HBV

hepatitis B virus

NLS

nuclear localization sequence

NP

nucleoplasmin

NPC

nuclear pore complex

Footnotes

REFERENCES

1. Akey CW, Radermacher M. Architecture of the Xenopus nuclear pore complex revealed by three-dimensional cryo-electron microscopy. J Cell Biol. 1993;122:1–19. doi: 10.1083/jcb.122.1.1. [DOI] [PMC free article] [PubMed] [Google Scholar]
2. Baschong W, Wrigley NG. Small colloidal gold conjugated to Fab fragments or to immunoglobulin G as high-resolution labels for electron microscopy: a technical overview. J Electron Microsc Tech. 1990;14:313–323. doi: 10.1002/jemt.1060140405. [DOI] [PubMed] [Google Scholar]
3. Catimel B, Teh T, Fontes MR, Jennings IG, Jans DA, Howlett GJ, Nice EC, Kobe B. Biophysical characterization of interactions involving importin-alpha during nuclear import. J Biol Chem. 2001;276:34189–34198. doi: 10.1074/jbc.M103531200. [DOI] [PubMed] [Google Scholar]
4. Chook YM, Cingolani G, Conti E, Stewart M, Vetter I, Wittinghofer A. Pictures in cell biology. Structures of nuclear-transport components. Trends Cell Biol. 1999;9:310–311. doi: 10.1016/s0962-8924(99)01610-4. [DOI] [PubMed] [Google Scholar]
5. Cingolani G, Petosa C, Weis K, Muller CW. Structure of importin-beta bound to the IBB domain of importin-alpha. Nature. 1999;399:221–229. doi: 10.1038/20367. [DOI] [PubMed] [Google Scholar]
6. Conti E, Izaurralde E. Nucleocytoplasmic transport enters the atomic age. Curr Opin Cell Biol. 2001;13:310–319. doi: 10.1016/s0955-0674(00)00213-1. [DOI] [PubMed] [Google Scholar]
7. Conti E, Uy M, Leighton L, Blobel G, Kuriyan J. Crystallographic analysis of the recognition of a nuclear localization signal by the nuclear import factor karyopherin alpha. Cell. 1998;94:193–204. doi: 10.1016/s0092-8674(00)81419-1. [DOI] [PubMed] [Google Scholar]
8. Crowther RA, Kiselev NA, Bottcher B, Berriman JA, Borisova GP, Ose V, Pumpens P. Three-dimensional structure of hepatitis B virus core particles determined by electron cryomicroscopy. Cell. 1994;77:943–950. doi: 10.1016/0092-8674(94)90142-2. [DOI] [PubMed] [Google Scholar]
9. De Robertis EM, Longthorne RF, Gurdon JB. Intracellular migration of nuclear proteins in Xenopus oocytes. Nature. 1978;272:254–256. doi: 10.1038/272254a0. [DOI] [PubMed] [Google Scholar]
10. Dingwall C, Sharnick SV, Laskey RA. A polypeptide domain that specifies migration of nucleoplasmin into the nucleus. Cell. 1982;30:449–458. doi: 10.1016/0092-8674(82)90242-2. [DOI] [PubMed] [Google Scholar]
11. Dworetzky SI, Lanford RE, Feldherr CM. The effects of variations in the number and sequence of targeting signals on nuclear uptake. J Cell Biol. 1988;107:1279–1287. doi: 10.1083/jcb.107.4.1279. [DOI] [PMC free article] [PubMed] [Google Scholar]
12. Feldherr CM, Kallenbach E, Schultz N. Movement of a karyophilic protein through the nuclear pores of oocytes. J Cell Biol. 1984;99:2216–2222. doi: 10.1083/jcb.99.6.2216. [DOI] [PMC free article] [PubMed] [Google Scholar]
13. Frens G. Controlled nucleation for the regulation of the particle size in minodisperse gold suspension. Nature. 1973;241:20–22. [Google Scholar]
14. Görlich D, Prehn S, Laskey RA, Hartmann E. Isolation of a protein that is essential for the first step of nuclear import. Cell. 1994;79:767–778. doi: 10.1016/0092-8674(94)90067-1. [DOI] [PubMed] [Google Scholar]
15. Görlich D, Kostka S, Kraft R, Dingwall C, Laskey RA, Hartmann E, Prehn S. Two different subunits of importin cooperate to recognize nuclear localization signals and bind them to the nuclear envelope. Curr Biol. 1995;5:383–392. doi: 10.1016/s0960-9822(95)00079-0. [DOI] [PubMed] [Google Scholar]
16. Hinshaw JE, Carragher BO, Milligan RA. Architecture and design of the nuclear pore complex. Cell. 1992;69:1133–1141. doi: 10.1016/0092-8674(92)90635-p. [DOI] [PubMed] [Google Scholar]
17. Horisberger M, Rosset J. Colloidal gold, a useful marker for transmission and scanning electron microscopy. J Histochem Cytochem. 1977;25:295–305. doi: 10.1177/25.4.323352. [DOI] [PubMed] [Google Scholar]
18. Kann M, Gerlich WH. Effect of core protein phosphorylation by protein kinase C on encapsidation of RNA with core particles of hepatitis B virus. J Virol. 1994;68:7993–8000. doi: 10.1128/jvi.68.12.7993-8000.1994. [DOI] [PMC free article] [PubMed] [Google Scholar]
19. Kann M, Bischof A, Gerlich WH. In vitro model for the nuclear transport of the hepadnavirus genome. J Virol. 1997;71:1310–1316. doi: 10.1128/jvi.71.2.1310-1316.1997. [DOI] [PMC free article] [PubMed] [Google Scholar]
20. Kann M, Sodeik B, Vlachou A, Gerlich WH, Helenius A. Phosphorylation-dependent binding of hepatitis B virus core particles to the nuclear pore complex. J Cell Biol. 1999;145:45–55. doi: 10.1083/jcb.145.1.45. [DOI] [PMC free article] [PubMed] [Google Scholar]
21. Kasamatsu H, Nakanishi A. How do animal DNA viruses get to the nucleus? Annu Rev Microbiol. 1998;52:627–686. doi: 10.1146/annurev.micro.52.1.627. [DOI] [PubMed] [Google Scholar]
22. Kenney JM, von Bonsdorff CH, Nassal M, Fuller SD. Evolutionary conservation in the hepatitis B virus core structure: comparison of human and duck cores. Structure. 1995;3:1009–1019. doi: 10.1016/s0969-2126(01)00237-4. [DOI] [PubMed] [Google Scholar]
23. Leunissen JL, De May JR. Preparation of gold probes. In: Verkleij AJ, Leunissen JL, editors. Immuno Gold Labeling. Boca Raton, FL: CRC Press; 1989. pp. 3–16. [Google Scholar]
24. Mattaj IW, Englmeier L. Nucleocytoplasmic transport the soluble phase. Annu Rev Biochem. 1998;67:265–306. doi: 10.1146/annurev.biochem.67.1.265. [DOI] [PubMed] [Google Scholar]
25. Moroianu J, Blobel G, Radu A. Previously identified protein of uncertain function is karyopherin alpha and together with karyopherin beta docks import substrate at nuclear pore complexes. Proc Natl Acad Sci USA. 1995;92:2008–2011. doi: 10.1073/pnas.92.6.2008. [DOI] [PMC free article] [PubMed] [Google Scholar]
26. Nakielny S, Dreyfuss G. Transport of proteins and RNAs in and out of the nucleus. Cell. 1999;23:677–690. doi: 10.1016/s0092-8674(00)81666-9. [DOI] [PubMed] [Google Scholar]
27. Paine PL, Moore LC, Horowitz SB. Nuclear envelope permeability. Nature. 1975;254:109–114. doi: 10.1038/254109a0. [DOI] [PubMed] [Google Scholar]
28. Panté N, Aebi U. The nuclear pore complex. J Cell Biol. 1993;122:977–984. doi: 10.1083/jcb.122.5.977. [DOI] [PMC free article] [PubMed] [Google Scholar]
29. Panté N, Aebi U. Towards understanding the 3-D structure of the nuclear pore complex at the molecular level. Curr Opin Struct Biol. 1994;4:187–196. [Google Scholar]
30. Panté N, Jarmolowski A, Izaurralde E, Sauder U, Baschong W, Mattaj IW. Visualizing nuclear export of different classes of RNA by electron microscopy. RNA. 1997;3:498–513. [PMC free article] [PubMed] [Google Scholar]
31. Radu A, Blobel G, Moore MS. Identification of a protein complex that is required for nuclear protein import and mediates docking of import substrate to distinct nucleoporins. Proc Natl Acad Sci USA. 1995;92:1769–1773. doi: 10.1073/pnas.92.5.1769. [DOI] [PMC free article] [PubMed] [Google Scholar]
32. Ribbeck K, Görlich D. Kinetic analysis of translocation through nuclear pore complexes. EMBO J. 2001;20:1320–1330. doi: 10.1093/emboj/20.6.1320. [DOI] [PMC free article] [PubMed] [Google Scholar]
33. Richardson WD, Mills AD, Dilworth SM, Laskey RA, Dingwall C. Nuclear protein migration involves two steps: rapid binding at the nuclear envelope followed by slower translocation through nuclear pores. Cell. 1988;52:655–664. doi: 10.1016/0092-8674(88)90403-5. [DOI] [PubMed] [Google Scholar]
34. Slot JW, Geuze HJ. A new method of preparing gold probes for multiple-labeling cytochemistry. Eur J Cell Biol. 1985;38:87–93. [PubMed] [Google Scholar]
35. Stoffler D, Fahrenkrog B, Aebi U. The nuclear pore complex: from the architecture to functional dynamics. Curr Opin Cell Biol. 1999;11:391–401. doi: 10.1016/S0955-0674(99)80055-6. [DOI] [PubMed] [Google Scholar]
36. Wente SR. Gatekeepers of the nucleus. Science. 2000;288:1374–1377. doi: 10.1126/science.288.5470.1374. [DOI] [PubMed] [Google Scholar]
37. Whittaker GR, Helenius A. Nuclear import and export of viruses and virus genomes. Virology. 1998;246:1–23. doi: 10.1006/viro.1998.9165. [DOI] [PubMed] [Google Scholar]
38. Whittaker GR, Kann M, Helenius A. Viral entry into the nucleus. Annu Rev Cell Dev Biol. 2000;16:627–651. doi: 10.1146/annurev.cellbio.16.1.627. [DOI] [PubMed] [Google Scholar]
39. Wrigley NG. The lattice spacing of crystalline catalase as an internal standard of length in electron microscopy. J Ultrastruct Res. 1968;24:454–464. doi: 10.1016/s0022-5320(68)80048-6. [DOI] [PubMed] [Google Scholar]