Cellular prion protein status in sheep: tissue-specific ... - CiteSeerX

Journal of General Virology (2001), 82, 2017–2024. Printed in Great Britain ...................................................................................................................................................................................................................................................................................

Cellular prion protein status in sheep : tissue-specific biochemical signatures Mohammed Moudjou,1 Yveline Frobert,2 Jacques Grassi2 and Claude La Bonnardie' re1 1 2

Institut National de la Recherche Agronomique (INRA) Virologie et Immunologie Mole! culaires, 78352 Jouy en Josas, France Unite! de Pharmacologie et d ’Immunologie, CEA Saclay, Gif/Yvette, France

Expression of the cellular prion protein PrPC is sine qua none for the development of transmissible spongiform encephalopathy and thus for the accumulation of the illness-associated conformer PrPSc. Therefore, the tissue distribution of PrPC at the protein level in both quantitative and qualitative terms was investigated. PrPC was quantified using a two-site enzyme immunometric assay which was calibrated with purified ovine recombinant prion protein (rPrP). The most PrPC-rich tissue was the brain, followed by the lungs, skeletal muscle, heart, uterus, thymus and tongue, which contained between 20- and 50-fold less PrPC than the brain. The PrPC content of these tissues seems to be comparable between sheep. Other organs, however, showed different, but low, levels of the protein depending on the animal examined. This was also the case for tissues from the gastrointestinal tract. The tissue containing the lowest concentration of PrPC was shown to be the liver, where PrPC was found to be between 564- and 16 000-fold less abundant than in the brain. PrPC was concentrated from crude cellular extracts by immunoprecipitation using several monoclonal and polyclonal anti-ovine PrP antibodies. Interestingly, it was observed that the isoform profile of PrPC was tissue-specific. The most atypical electrophoretic profile of PrPC was found in the skeletal muscle, where two polypeptides of 32 and 35 kDa were detected.

Introduction Prion diseases belong to a family of neurodegenerative disorders that affect both humans and animals. The mechanisms of prion transmission are not yet unravelled. Nevertheless, it is admitted today that one of the fundamental steps in pathogenesis is the conversion of the host-encoded cellular prion protein PrPC into its disease-associated conformer PrPSc (Prusiner, 1998 ; Jackson & Clarke, 2000). Transmissible spongiform encephalopathies (TSE) are characterized by an accumulation of PrPSc in the brain and the expression of PrPC has been shown to be crucial for the transmission of the disease and formation of PrPSc (Bu$ eler et al., 1993 ; Prusiner et al., 1993 ; Weissmann, 1996). One of the emerging hypotheses is that the conversion phenomenon could take place at the site where the infectious agent meets PrPC. The latter has been shown to be expressed in various domains of the hamster brain (Bendheim et al., 1992 ; DeArmond et al., 1999 ; Somerville, 1999) and in several non-neuronal tissues from rodents (Bendheim et al., 1992), cows and humans, including the spleen Author for correspondence : Mohammed Moudjou. Fax j33 1 34 65 26 21. e-mail moudjou!biotec.jouy.inra.fr

0001-7776 # 2001 SGM

and lymph nodes (McBride et al., 1992), squamous epithelia of the skin and upper gastrointestinal tract (Pammer et al., 1998, 1999). PrPC has also been detected on the surface of lymphocytes in humans and mice (Cashman et al., 1990 ; Mabbott et al., 1997 ; Antoine et al., 2000). A PrP isoform truncated at the C terminus has been detected in mature human and bovine sperm (Shaked et al., 1999). In addition, PrPC mRNA has been shown to be present in all tissues tested to date from humans, cattle and sheep (Goldmann et al., 1999). Nevertheless, precise qualitative and quantitative studies of PrPC expression at the protein level have never been carried out in sheep. The difficulties for such an investigation are principally due to the lack of efficient and sensitive methods to concentrate, detect and quantify PrPC from non-neuronal tissues, in which its expression is expected to be low. Horiuchi et al. (1995) made the first determination of PrPC distribution in sheep organs and showed that PrPC can be detected in several tissues other than the brain. The ratio between PrPC expression in the brain and other tissues could not, however, be precisely determined at that time. Here we report the first quantification of PrPC in different tissues of sheep using a two-site enzyme immunometric assay (EIA). Furthermore, by use of a simple method to immunoCABH

M. Moudjou and others

precipitate PrPC from a crude tissue extract of healthy sheep tissue, we have demonstrated that the isoform profile of PrPC is tissue-specific. The most striking PrPC glycoform profile was obtained from skeletal muscle.

Methods

Antibodies. The anti-PrP monoclonal antibodies (MAbs) used in the present work were 4F2 and 12F10 (Krasemann et al., 1996), which were obtained from Le Re! seau Anticorps du Programme Français de Recherche sur les ESST, and SAF34 and SAF37, which were produced using hamster scrapie-associated fibrils as the immunogen and present a 4F2-like specificity (octarepeat region) (Rodolfo et al., 2001). Pc248 was obtained after immunization of PrP−/− mice with PrPC purified from sheep brain (unpublished data). The anti-PrP polyclonal antibody (PAb) MH44 was obtained after immunization of rabbits with ovine recombinant PrP (rPrP) expressed in Escherichia coli and purified to homogeneity by virtue of its intrinsic capacity to bind some divalent cations (Rezaei et al., 2000). Specific peroxidase-conjugated anti-rabbit immunoglobulins (IgGs) were purchased from BioSys.

Tissue preparation. Seven 2-year-old ewes (ewe I, PrnP genotype ARQ\ARR at positions 136, 154 and 171 ; ewe II, ARQ\ARR ; ewe III, ARQ\ARR ; ewe IV, ARQ\VRQ ; ewe V, AHQ\ARR ; ewe VI, ARQ\ARR ; and ewe VII, ARQ\ARR) in the early stages of pregnancy were sacrificed under controlled conditions and the organs were rapidly removed and placed on ice for a maximum of 30 min. After washing with PBS, each organ was frozen at k80 mC until use. The genotype at the PrnP locus was determined for codons 136, 154 and 171 at Labogena, as described by Elsen et al. (1999) except that DNA was purified from skeletal muscle tissues.

Tissue extraction. One sample of each sheep organ was homogenized to a 10 % suspension with a Polytron homogenizer (Kinematica) in two different extraction buffers : buffer B (12n5 mM Tris, 12n5 mM MES, pH 6n8, 50 mM NaCl, 1 % Zwittergent 3-12) ; or TL1 buffer (50 mM Tris–HCl, pH 7n5, 0n5 % Triton X-100, 0n5 % deoxycholate). Both buffers contained 1 mM PMSF and 2 µg\ml each of aprotinin, leupeptin and pepstatin (Sigma) as protease inhibitors. After centrifuging the crude extract at 4 mC for 10 min at 4000 g, supernatants were removed and processed.

Quantification of PrPC in different tissues using a two-site EIA. The solid phase EIA technique used in the present work is described in detail by Rodolfo et al. (2001). Microtitre plates (Immunoplate Maxisorp, Nunc) were coated with the capture IgG MAbs SAF34 or SAF37. The plates were then saturated with EIA buffer (0n1 M potassiumphosphate buffer, pH 7n4, 0n15 M NaCl, 0n1 % BSA) and stored at 4 mC until use. Before use, the plates were washed three times with wash buffer (10 mM phosphate buffer, pH 7n4, containing 0n05 % Tween 20) and then processed for the EIA test. Ovine rPrP (VRQ allele), purified as described by Rezaei et al. (2000), was used as an internal plate control to produce a standard curve ranging from 10 to 0n078 ng\ml. Different dilutions of extracts corresponding to each tissue were made in EIA buffer containing 0n1 % Triton X-100 and processed at the same time as the standard protein. All dilutions were duplicated in each experiment. After 3 h of incubation at room temperature with mild shaking, the microtitre plates were washed three times with wash buffer and incubated overnight at 4 mC with the tracer antibody. The latter consists of Fabh fragments obtained from 12F10 IgGs and coupled to a G4 tetramer of acetylcholinesterase (AchE) (Grassi et al., 1988). After three washes, AchE CABI

activity was assessed by adding Ellman reagent (Ellman et al., 1961) and measuring absorbance at 414 nm with an automatic reader (LabSystems).

PrPC immunoprecipitation. Anti-PrP MAbs Pc248 or 4F2 were added to 500 µl (50 mg tissue equivalent) of the different clarified total extracts, obtained as described above. The samples were then incubated for 1 h at room temperature. To spin down the immunocomplexes, protein A–Sepharose beads (Pharmacia–Amersham) were added to the mixtures and incubated for 1 h at room temperature or overnight at 4 mC on a rotating wheel. The beads were then washed four times with the corresponding extraction buffer and once with double-distilled water before dissolving in 50 µl of 8 M urea and 20 mM DTT. The correct volume of 4i Laemmli sample buffer was then added (Laemmli, 1970).

Deglycosylation of PrPC. The immunoprecipitated PrPC present in the urea\Laemmli sample buffer was diluted in deglycosylation buffer (50 mM Tris–HCl, pH 8n0, 1 % Nonidet-P40) and treated with 0n5 U\ml of N-glycosidase F (Boehringer Mannheim) for 5 h at 37 mC. Samples were precipitated with 10 % trichloroacetic acid and washed twice with ethanol before dissolving in Laemmli sample buffer and analysis by Western blotting.

Analytical methods. SDS–PAGE was performed with the Miniprotean II Biorad system. Gel transfer of proteins separated by SDS–PAGE was carried out using the Minigel Transblot Cell system (Biorad), according to the manufacturer’s instructions. Low molecular mass markers (Pharmacia–Amersham) were as follows : phosphorylase b, 94 kDa ; BSA, 67 kDa ; ovalbumin, 43 kDa ; carbonic anhydrase, 30 kDa ; soybean trypsin inhibitor, 20 kDa ; and α-lactalbumin, 14 kDa. After immunoprecipitation with the anti-PrP MAbs Pc248 or 4F2, PrPC was detected using either the purified IgG fraction of MH44 PAb or the biotinylated 4F2 MAb. PrPC was then visualized using the ECL detection technique with specific goat anti-rabbit IgGs coupled to peroxidase or streptavidin-coupled peroxidase (Pierce), respectively. Protein content was determined by the Bradford method.

Results Quantification of PrPC in different tissues PrPC was quantified in crude tissue homogenates with a

sensitive quantification test for the prion protein (Rodolfo et al., 2001). In all cases, the quantification test was calibrated using ovine rPrP purified from E. coli. This allowed us to produce a reproducible linear standard curve with a detection limit of up to 2n5 ng\ml (data not shown ; Rodolfo et al., 2001). The standard curve was similar whether rPrP was diluted in ELISA buffer or in brain homogenate obtained from PrP−/− mice (Rodolfo et al., 2001). The detection limit obtained with the antibodies used in the present test is around 70 pg\ml. Two series of sheep were used to carry out this study. Fewer organs were removed from the first series (ewes I–III). The results for all sheep tested are presented as histograms in Figs 1 and 2. The overall distribution of PrPC in ewes I–III (ARQ\ARR) gave comparable values with only few exceptions (Fig. 1). Aside from the brain, the other tissues from these animals that contained significant amounts of PrPC were the lungs, heart and skeletal muscle, although in quantities of 20-, 36- and 34fold less than in the brain, respectively. Ewe IV (ARQ\VRQ) showed some difference in PrPC distribution compared with

Tissue distribution of sheep PrPC

content (between 0n3 and 4 ng\g of tissue) in all of the sheep tested. Tissue-specific isoform distribution of PrPC

Fig. 1. PrPC quantification in different tissues from ewes I–III. The PrPC content in the brain is expressed in µg/g of tissue, while it is in ng/g of tissue for the other organs. The different tissues tested were as follows : tonsil (Ts), tongue (Tg), lung (Lu), heart (H), liver (Li), spleen (Sp), pancreas (Pa), kidney (Ki) and skeletal muscle (SM).

that found in the same tissues from ewes I–III (Figs 1 and 2). PrPC content in the tonsils of ewe IV was, for example, about three to four times greater than that in ewes I and II. Furthermore, the lungs of ewe IV contained less PrPC than ewes I–III. The uterus was found to be the most PrPC-rich extraneuronal tissue in ewe IV. PrPC was also detected in the salivary glands of ewe V and in the mammary glands of ewe IV (Fig. 2). However, because of the limited number of sheep studied, no conclusion regarding genotype effects on the level of PrPC can be drawn at this stage. PrPC was quantified in different tissues taken from the digestive tract of ewes IV–VI. However, only values for ewes IV and V are shown (Fig. 2). PrPC was detected in all of the tissues tested. The values obtained for ewes V and VI along the digestive tract were, however, found to be two to four times less than what was quantified for ewe IV. Interestingly, we have observed that the liver is the tissue with the lowest PrPC

To check whether the organs differed only by their content of PrPC or, in addition, by the biochemical signature of the protein, we developed an immunoprecipitation method to concentrate PrPC from whole tissue extracts. All tissues were homogenized to the same wt\vol ratio (10 %). We first tried to detect PrPC by classical Western blot using several anti-PrP MAbs and PAbs. Only brain extract showed strong labelling of PrPC (data not shown). However, after lengthy exposure of the nitrocellulose membranes, we detected faint signals of PrPC, but always in the same tissues, in the skeletal muscle, tongue, lungs and heart (data not shown). We then decided to concentrate PrPC by immunoprecipitation directly from each clarified crude tissue extract before its detection by Western blot. Fig. 3 shows an example of a comparative immunoprecipitation experiment with both MAb Pc248 IgG1 and an anti-PrPC unrelated mouse IgG1 on the same tissue extracts from ewe VII. Only results obtained with extracts prepared in TL1 buffer are shown, as they gave the best results (especially from non-neuronal tissues). The control IgG did not immunoprecipitate PrPC from the different extracts (Fig. 3 C). PrPC was detected after immunoprecipitation with Pc248 using two different probes, PAb MH44 (Fig. 3 A), which was obtained after injection of ovine rPrP into rabbits and had been shown to specifically recognize PrPC in a crude brain homogenate from different species (data not shown), and biotinylated MAb 4F2 (Krasemann et al., 1996) (Fig. 3 B). In both cases, the same PrPC profile was obtained, although the intensity of PrPC bands differed slightly in a few tissues depending on the primary antibody used. Furthermore, pre-incubation of the primary antibodies used for Western blot with an excess of purified PrP abolished detection of the immunoprecipitated PrPC (data not shown). Altogether, these data showed that the signals obtained with Pc248 were specific for PrPC. In order to be confident with the results obtained with Pc248, we repeated the immunoprecipitation experiment with 4F2 (purified IgG) on the same tissue extracts. As shown in Fig. 4, the same kind of PrPC profile was obtained, irrespective of the Western blot detection probe used to visualize the immunoprecipitated PrPC (biotinylated 4F2 IgG, Fig. 4 A ; MH44 IgGs, Fig. 4 B). It is evident from the Western blots carried out after immunoprecipitation that several other non-neuronal tissues showed significant levels of PrPC. A striking tissue specificity in the qualitative profile of the different isoforms of PrPC was obtained. Actually, the glycoform signature of PrPC in the brain, as obtained with most anti-PrP antibodies described in the literature, is in general characterized by the presence of three bands with decreasing intensity, representing the bi-, CABJ


Fig. 2. An example of PrPC content in a sheep from which gastrointestinal tract tissues were studied (ewes IV and V). The different tissues tested were as follows : tonsil (Ts), tongue (Tg), lung (Lu), heart (H), liver (Li), spleen (Sp), pancreas (Pa), kidney (Ki), skeletal muscle (SM), uterus (Ut), thymus (Tm), reticulum (Re), rumen (Ru), duodenum (Du), jejunum (Je), ileum (IL), mammary glands (Ma) and salivary glands (SG). nd, Not detected.

mono- and unglycosylated isoforms of PrP (Fig. 4 C, lanes Br). In the lungs, a complex profile with hyperglycosylated isoforms was always observed. Furthermore, the band migrating at the level of the unglycosylated isoform from the lungs migrated slightly faster than its corresponding band from the brain (Figs 4 A, B and 5 A). The second atypical PrPC electrophoretic profile was reproducibly observed in skeletal muscle, where a clear doublet of PrPC was detected from all seven sheep tested (Figs 3 and 4, lanes SM). The PrPC profile of skeletal muscle was specific, since it was not observed in other types of muscular tissue, such as the heart and tongue. In the uterus, either with or without myometrium, the PrPC profile was different from that observed in skeletal muscle and was more reminiscent of the heart PrPC profile (data not shown). The two bands from skeletal muscle migrated slower than the bi- and monoglycosylated isoforms from the brain : 32 kDa in the skeletal muscle instead of 30 kDa in brain for the monoglycosylated band and 35 kDa in skeletal muscle instead of 33 kDa in brain for the biglycosylated band (Fig. 5). The signals obtained from the spleen and kidney were often very CACA

low (Figs 1–3). PrPC was not significantly detected from liver tissue (Figs 3 and 4). This indicates that liver tissue contains the lowest amount of PrPC, if any, within the detection limits of the immuno-concentration method described in the present work. Secondly, we investigated the distribution of PrPC along the digestive tract. Sections of tissue from the gastrointestinal tract were removed from the second series of sheep (ewes IV–VII). Only results from ewe VII are shown. We have observed that the signals obtained for PrPC from these tissues were often diffuse at the level of biglycosylated forms (Figs 3 and 4). The distribution of PrPC along the digestive tract was shown to be different from one sheep to another (Fig. 2). In ewe VII, PrPC was found all along the digestive tract, with more PrPC in the reticulum and ileum (Figs 3 and 4), whereas in ewe IV, PrPC was mainly detected in the reticulum, rumen and duodenum (Fig. 2). In ewe V, PrPC was concentrated in the reticulum and rumen (Fig. 2). In order to check that the PrPC isoforms detected in some tissues corresponded to glycoforms, we carried out a deglycosylation experiment on PrPC immunoprecipitated from


Discussion

Fig. 3. Immunoprecipitation (IP) of PrPC from different tissue extracts by both Pc248 anti-PrP MAb (A, B) and an anti-PrP unrelated control mouse IgG (C) analysed by Western blot (WB) with either MH44 anti-PrP IgG (A, C) or biotinylated 4F2 IgG (B). Tissues were taken from ewe VII. Asterisks indicate the PrPC doublet detected from skeletal muscle homogenate. The different tissues tested were as follows : brain (Br), tongue (Tg), tonsil (Ts), lung (Lu), heart (H), spleen (Sp), liver (Li), skeletal muscle (SM), reticulum (Re), rumen (Ru), duodenum (Du), jejunum (Je), ileum (IL), mammary glands (Ma) and pancreas (Pa). Lane Br1/4 shows a fourth dilution of the PrPC fraction obtained from brain to distinguish the three PrPC glycoforms.

the skeletal muscle, lung and brain (Fig. 5). Treatment of PrPC with N-glycosidase F resulted in simplifying the PrPC profile into one band, which probably corresponds to nonglycosylated PrPC (Fig. 5). Interestingly the nonglycosylated PrPC isoform obtained from the lung migrated faster than those obtained from the brain and skeletal muscle.

PrPC expression is necessary for the development of TSE (Bu$ eler et al., 1993 ; Prusiner et al., 1993). The spatial sequence of events after oral infection is still not completely understood. Following oral challenge, it is assumed that the gastrointestinal tract and its associated lymphoreticular system represent the first tissues in which PrPSc could be detected, thus corresponding to tissues that support infection (McKinley et al., 1983 ; Race et al., 1998 ; van Keulen et al., 1999 ; Bons et al., 1999 ; Maignien et al., 1999 ; Beekes & McBride, 2000 ; Andre! oletti et al., 2000). PrPC has been found to be the substrate for the formation of its pathology-associated conformer PrPSc (Weissmann, 1996). The distribution of the cellular form, PrPC, in non-neuronal tissues is not, however, well documented in sheep. The quantification test used in the present work permitted the PrPC ratio between the brain and the extraneuronal tissues to be determined. The EIA test was able to detect PrPC in several crude non-neuronal tissue extracts, even after a tenfold dilution. We should mention here that the EIA was originally designed to detect PrPres for the post-mortem diagnosis of bovine spongiform encephalopathy. In this context, the EIA was evaluated by the European Commission, supervised by the Directorate XXIV (Moynagh & Schimmel, 1999 ; Moynagh et al., 1999) and it was concluded that this test was ‘ the most sensitive one ’ at that time. In general, there was a good correlation between the results obtained with the EIA and those observed using the immunoprecipitation\Western blot experiment. The tissue distribution of PrPC in sheep was first studied by Horiushi et al. (1995). However, Horiushi and co-workers used microsomal preparations from different tissues to enrich PrPC. We have recently shown that the solubilized microsomal PrPC population correspond to 16 % of total brain PrPC only (unpublished data). Altogether, these data prompted us to set up a different procedure which could better reflect the true PrPC content of different tissues in both qualitative and quantitative terms. In all cases, PrPC could be detected by loading only 5 mg of tissue equivalent per lane from almost all tissues except the liver. Serial dilutions made from the tissues richest in PrPC content (lungs, skeletal muscle and heart) showed that we could still detect PrPC in an equivalent of 0n5 to 1 mg of tissue (data not shown). Similar results were obtained from immunoprecipitation\ Western blot assays using several combinations of MAbs and PAbs. Furthermore, we have observed that two different antiPrP PAbs, MH44 and MH48, produced in our laboratory immunoprecipitated an additional faint band of about 66 kDa from skeletal muscle (data not shown). This band could correspond to a dimeric form of PrPC which is present specifically in this tissue. Comparable results from different animals were found in several tissues, such as the lungs, heart, skeletal muscle and tongue. Data from the gastrointestinal tract CACB


Fig. 4. PrPC distribution in different tissues from ewe VII using 4F2 IgG for immunoprecipitation (IP) followed by Western blot (WB) detection with either biotinylated 4F2 IgG (A) or MH44 anti-PrP PAb IgG (B). The different tissues tested were as follows : brain (Br), tongue (Tg), tonsil (Ts), lung (Lu), heart (H), spleen (Sp), liver (Li), skeletal muscle (SM), reticulum (Re), rumen (Ru), duodenum (Du), jejunum (Je), ileum (IL) and mammary glands (Ma). (C) IP of PrPC from H, SM and Br samples from ewes III and II, indicating the specific muscle profile of PrPC. Note the difference in migration between the bi- and monoglycosylated isoforms of brain PrPC and the PrPC doublet observed in SM. Bi-, mono- and nonglycosylated (B, M and N) isoforms described in the brain are indicated on the right.

A

B

Fig. 5. Sensitivity of PrPC from the brain, skeletal muscle and lungs to treatment with N-glycosidase F. PrPC immunoprecipitated with MAb 4F2 from the brain (Br), skeletal muscle (SM) and lung (Lu) extracts were either (A) untreated (kPNGase) or (B) incubated with N-glycosidase F (jPNGase), as described in Methods. PrPC was detected by Western blotting with biotinylated 4F2 MAb. Lanes SM and Lu were loaded with PrPC immunoprecipitated from the same amount of tissue extract, while lane Br represents PrPC obtained from a third tissue equivalent of brain than skeletal muscle and lungs. Note that the nonglycosylated PrPC isoform in the lungs migrated with a reduced molecular mass.

tissues varied between individual sheep. Given the low number of sheep tested in the present work, we could not determine whether there is any relationship between animal genotype for the PrP locus and the tissue expression of PrPC. Interestingly, in all organs from which PrPC could be immunoprecipitated, bands of either bi- or hyperglycosylated isoforms were clearly detected. Nevertheless, a specific PrPC isoform signature was systematically observed in the skeletal muscle (from either the thigh or the flank) : two bands migrating more slowly than the CACC

brain mono- and biglycosylated isoforms (Fig. 5). These two bands correspond to PrPC glycoforms, as deglycosylation resulted in one band migrating at the same level as that of the nonglycosylated protein obtained from the brain. However, differences in the composition and length of the oligosaccharide chains present on PrPC could differ in the brain and skeletal muscle, and this could explain the difference in migration observed between the mono- and biglycosylated isoforms from these two tissues. Furthermore, we have shown that the nonglycosylated form obtained from the lungs migrated faster than its equivalents from the brain and skeletal muscle. Whether this is the result of N- or C-terminal truncation is not yet known. Indeed, a PrP isoform truncated at the Cterminal has been observed in mature human and bovine sperm (Shaked et al., 1999). We should note here that pieces of skeletal muscle were removed with careful attention to avoid any residual nervous fibres. However, some neuromuscular junctions probably remained. Several arguments indicate that the typical muscular profile described here really belongs to muscle cells. PrPC has indeed been detected in developing mouse muscle cells (Brown et al., 1998). Furthermore, PrPC has been immunolocalized at the subsynaptic sarcoplasm of the neuromuscular junction of mammalian muscles (Gohel et al., 1999 ; Askanas et al., 1993). PrPC has also been detected by immunoblotting in skeletal muscle from hamster (Bendheim et al., 1992) and in quadriceps muscle homogenates from non-transgenic mice (Westaway et al., 1994). Overexpression of hamster PrPC in homozygote Tg(ShaPrP+/+)7 uninfected older mice resulted in spontaneous degeneration of the central nervous system (CNS) and skeletal muscle neuromyopathy (Westaway et al., 1994). Altogether,


these results underline a potential role of PrPC in skeletal muscle cells. The tissue distribution and developmental expression of sheep PrP mRNA has been published by Goldmann et al. (1999). No correlation between mRNA and protein levels can, however, be established. Altogether, these data reflect either a tissue-specific regulation of mRNA initiation, translation and\or stability, or a tissue-specific PrPC catabolism control. Our finding supports the idea that organs for which infectivity has been demonstrated (tonsil, thymus, intestine and spleen) do not contain more PrPC than tissues shown not to support infection (skeletal muscle and heart) (Hadlow et al., 1979 ; Danner, 1993). Thus, like the ‘ species barrier ’, a ‘ tissue barrier ’ phenomenon for infection might also exist. Several hypotheses could be proposed : (i) it is possible that physical and\or physiological barriers may preclude the infectious agent from reaching some tissues, (ii) the existence of cofactors necessary for the achievement of PrPC conversion in tissues that support infection or the presence of inhibitory molecules in uninfectious organs could also explain this discrepancy, and (iii) a possible relationship between the biochemical features of PrPC (e.g. glycoform diversity among tissues, unidentified tissue-specific PrPC post-translational modifications and tissue differences in PrP clearance) and its susceptibility to be converted into the scrapie form still remains an open question. One of the intriguing phenomena in sheep is the dependence on the PrnP locus genotype for susceptibility to scrapie (Bossers et al., 1996 ; Hunter et al., 1996). It has been demonstrated that animals which are highly susceptible to scrapie (homozygote VRQ\VRQ at positions 136, 154 and 171) accumulate PrPSc in the lymphoid tissue at early stages of the disease (Schreuder et al., 1996, 1998 ; van Keulen et al., 1996 ; Andre! oletti et al., 2000). Later on, PrPSc is detected in the CNS. This sequence of PrPSc appearance is not found in sheep that are moderately susceptible to scrapie (heterozygote ARR\VRQ), where PrPSc deposits are observed only in the CNS. These results indicate that the nature of the protein itself might play the role of a ‘ physiological bolt ’ to control the conversion events. In conclusion, the development of such biochemical and quantitative studies for tissue distribution of PrPC might allow important advances in understanding the biochemistry and function of this protein. Furthermore, these studies should be combined with the immunocytochemical localization of PrPC. The latter point will precisely indicate which cell type expresses PrPC in a given organ. It will be interesting then to look at the accumulation of PrPSc at the cellular level during the course of infection. This might aid the development of other pre-clinical diagnoses for TSE. We thank H. Rezaei and J. Grosclaude for providing us with recombinant ovine PrP ; E. Treguer, S. Labiau and M. Cluzeaud for Pc248 MAb production ; C. Cre! minon and P. Fre! tier for helpful advice with ELISA experimentation. We also thank H. Laude and D. Vilette for

helpful discussion, and Wendy Brand-Williams for checking the English. This work was supported by INRA and by Le Re! seau Français de Recherche sur les ESST.

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Received 3 April 2001 ; Accepted 8 May 2001 Published ahead of print (16 May 2001) in JGV Direct as DOI 10.1099/vir.0.17776-0