Advertisement
JBC

HOME HELP FEEDBACK SUBSCRIPTIONS ARCHIVE SEARCH TABLE OF CONTENTS
QUICK SEARCH:   [advanced]


     

Originally published In Press as doi:10.1074/jbc.M304449200 on July 16, 2003

J. Biol. Chem., Vol. 278, Issue 39, 37306-37313, September 26, 2003
This Article
Right arrow Abstract Freely available
Right arrow Full Text (PDF)
Right arrow All Versions of this Article:
278/39/37306    most recent
M304449200v1
Right arrow Submit a Letter to Editor
Right arrow Alert me when this article is cited
Right arrow Alert me when eLetters are posted
Right arrow Alert me if a correction is posted
Right arrow Citation Map
Services
Right arrow Email this article to a friend
Right arrow Similar articles in this journal
Right arrow Similar articles in PubMed
Right arrow Alert me to new issues of the journal
Right arrow Download to citation manager
Right arrowRequest Permissions
Citing Articles
Right arrow Citing Articles via Google Scholar
Google Scholar
Right arrow Articles by Baars, S.
Right arrow Articles by Rösl, F.
Right arrow Search for Related Content
PubMed
Right arrow PubMed Citation
Right arrow Articles by Baars, S.
Right arrow Articles by Rösl, F.
Social Bookmarking
Add to CiteULike   Add to Complore   Add to Connotea   Add to Del.icio.us   Add to Digg   Add to Reddit   Add to Technorati  
What's this?

Tyrphostin AG 555 Inhibits Bovine Papillomavirus Transcription by Changing the Ratio between E2 Transactivator/Repressor Function*

Sabine Baars {ddagger}, Anastasia Bachmann {ddagger}, Alexander Levitzki § and Frank Rösl {ddagger} 

From the {ddagger}Angewandte Tumorvirologie, Abteilung Virale Transformationsmechanismen, Deutsches Krebsforschungszentrum, Im Neuenheimer Feld 242, Heidelberg 69120, Germany and the §Department of Biological Chemistry, The Hebrew University, 91904 Jerusalem, Israel

Received for publication, April 29, 2003 , and in revised form, June 26, 2003.


   ABSTRACT
TOP
 ABSTRACT
INTRODUCTION
 EXPERIMENTAL PROCEDURES
 RESULTS
 DISCUSSION
 REFERENCES
 
The tyrosine kinase inhibitor (tyrphostin) AG 555 selectively interferes with viral transcription in bovine papillomavirus type 1 (BPV-1)-transformed fibroblasts and induces suppression of cyclin-dependent kinase activity and cell cycle arrest. Concomitant with inhibition of viral transcription, c-Jun was strongly up-regulated, which was consistent with the observation that AG 555 treatment also led to an activation of the mitogen-activated protein kinase pathway by enhancing phosphorylation of JNK and p38. Increased JNK and p38 activity resulted in higher phosphorylation of the AP-1 family members c-Jun and activating transcription factor 2. Scanning the BPV-1 genome for potential binding sequences, an intragenic AP-1 site (BAP-1) within the E7 open reading frame was detected. Enhanced dimerization of phosphorylated activating transcription factor 2 together with c-Jun and binding to BAP-1 seem to be responsible for viral dysregulation because both suppression of BPV-1 and induction of c-Jun mRNA could be almost entirely abrogated by simultaneous treatment with SB 203580, an inhibitor of p38 mitogen-activated protein kinase activity. Moreover, dissecting the complex transcriptional pattern of episomal BPV-1 with specific primer sets for reverse transcription-PCR analysis, the repressive effect could be attributed to a selective down-regulation of the mRNA encoding the E2 transactivator function in favor of the E2 repressor, whose mRNA level remained constant during AG 555 treatment. These data indicate that tyrphostin AG 555 disturbs the balance of negative and positive regulatory factors necessary to maintain the homeostasis of a virus-transformed phenotype.


   INTRODUCTION
TOP
 ABSTRACT
 INTRODUCTION
EXPERIMENTAL PROCEDURES
 RESULTS
 DISCUSSION
 REFERENCES
 
Increased tyrosine phosphorylation is a common feature of many cancers (1, 2). Up-regulation of specific receptors or/and enhanced tyrosine kinase activity concomitantly elevate intracellular phosphorylation of many downstream regulatory proteins, which guarantees the maintenance of unscheduled DNA synthesis and cell proliferation (for review, see Ref. 3). In recent years, defined synthetic compounds have been designed which can efficiently block tyrosine kinase activity (tyrphostins) (4) and in turn the proliferative phenotype. In principle, two types of tyrphostin have been developed: one is acting at the substrate binding site of the enzyme, whereas the other functions by competing with the ATP binding domain, which is highly conserved among tyrosine kinases (1). Tyrphostins structurally resemble tyrosine and erbstatin moieties and carry hydrophobic residues that enable crossing the cell membrane. The potential application of tyrphostins is not only considered for treatment of malignant disorders but also in other diseases such as atherosclerosis, psoriasis, and septic shock where increased tyrosine kinase activity could be discerned (5, 6). Furthermore, tyrphostins are also useful tools to study regulatory mechanisms where enhanced tyrosine phosphorylation is involved (2).

In the case of papillomavirus-linked diseases, alterations of epidermal growth factor (EGF)1/insulin-like growth factor I (IGF-I) signal transduction and in turn increased tyrosine phosphorylation seem to play a pivotal role during multistep progression toward malignancy (7–9). For example, the bovine papillomavirus type 1 (BPV-1) E5 oncoprotein exerts its transforming function through constitutive activation of growth stimulatory pathways via interaction with platelet-derived growth factor and EGF receptors (10, 11). Furthermore, both BPV-1 E5 and the corresponding homolog of the human papillomavirus (HPV) type 16 can cooperate with ectopic EGF receptor expression in cell transformation assays (12, 13). Although the E5 open reading frame (ORF) of HPV-16 is often found to be deleted in cervical carcinoma cells after integration (14), the protein may have a function in premalignant lesions (15), in which the DNA is still episomal (16). Intriguing also is the observation that rodent cells harboring a targeted disruption of the IGF receptor gene (IGF-R1) cannot be transformed by BPV-1 unless a functional IGF-R1 cDNA is provided (8). This supports the notion that enhanced tyrosine kinase activity is apparently a general feature in viral carcinogenesis because elevated expression of EGF/IGF receptors has been reported in a wide proportion of papillomavirus-induced malignancies (17, 18).

A suitable model system, in which enhanced intracellular tyrosine phosphorylation signaling can be studied in the context of viral transcription and transformation, is provided by BPV-1-transformed mouse fibroblasts (ID13 cells) (19). Here, E5 is considered the main oncoprotein (20) because mutations within the ORFs of E6 and E7 (encoding the major HPV-16/18-transforming proteins) (for review, see Ref. 21) have only marginal effects in focus formation assays using rodent cells as recipients (22). However, E6 can also affect tyrosine phosphorylation by interacting with the focal adhesion protein paxillin, known to be involved in coordination of cell spreading and motility (23). Similar to premalignant HPV-positive keratinocytes (24), BPV-1 persists as multicopy episomal nucleoprotein complexes in transformed cells (25, 26). This has the advantage that effects on the multipromoter-driven transcriptional activity (27, 28) can be investigated independently from any position effects (25) often occurring after viral integration into the host genome (29).

In the present study, we show that the tyrphostin AG 555 can selectively suppress BPV-1 transcription through MAP kinase pathway activation and binding of phosphorylated Jun/ATF-2 at a novel intragenic regulatory sequence. We also demonstrate that AG 555 affects the transcription of the major regulatory viral protein E2 by shifting the ratio between E2 transactivator in favor to the repressor function. These data indicate that fine tuning of BPV-1 gene expression in transformed cells is regulated by tyrosine phosphorylation.


   EXPERIMENTAL PROCEDURES
TOP
 ABSTRACT
 INTRODUCTION
 EXPERIMENTAL PROCEDURES
RESULTS
 DISCUSSION
 REFERENCES
 
Cell Culture and Treatment—ID13 mouse fibroblasts (19) were maintained in Dulbecco's modified Eagle's medium (Sigma) supplemented with 5% (v/v) fetal calf serum (Invitrogen), 100 units/ml penicillin, and 100 µg/ml streptomycin (Sigma). Cells were seeded at 2.5 x 104 cells/cm2 to ensure logarithmic growth. The final concentration of the tyrphostin AG 555 (cyano-3-(3,4-dihydroxyphenyl)-N-(3-phenylpropyl)-2-propenamide) was 30 µM in all experiments. Stock solutions of 10 mM in Me2SO were stored at –80 °C. To exclude potential Me2SO effects, the same final concentrations (0.3%) of Me2SO were added to nontreated controls. Actinomycin D (Calbiochem) was dissolved in water and added to cells in a final concentration of 5 µg/ml. SB 203580 (Calbiochem) was dissolved in Me2SO (stock concentration: 50 mM) and used in a final concentration of 10 µM.

Northern Blot Analysis—RNA was extracted according to the guanidinium-thiocyanate protocol described by Chomczynski and Sacchi (30). Approximately 5 µg of total cellular RNA was separated on 1% agarose gels (31) and transferred to GeneScreen Plus membranes (PerkinElmer Life Sciences). The filters subsequently were hybridized with specific DNA probes that were labeled with [32P]dCTP by random priming (32).

DNA Probes—pBPV-1 represents a unit length of BPV-1 DNA (33) cloned in pBR322. c-Jun, encoding the mouse cDNA in a Rous sarcoma virus-driven vector, was kindly obtained from Peter Angel, Deutsches Krebsforschungszentrum Heidelberg (34). pHF-{beta} A1 (35), harboring an approximately full-length insert of the fibroblast {beta}-actin gene, was a generous gift from L. Kedes (Medical Center, Palo Alto, CA).

Electrophoretic Mobility Shift Assays (EMSAs)—For gel retardation and competition assays, the following oligonucleotides were used: AP-1 consensus sequence, 5'-CGCTTGATGACTCAGCCGGAA-3'; TRE consensus sequence, 5'-AGCTAAAGTGGTGACTCATCACTAT-3' derived from the collagenase 3-/matrix metalloprotease 13 promoter) (34); SP-1 binding sequence: 5'-ATTCGATCGGGGCGGGGCGAGC-3', derived from the SV 40 promoter (36); and the BPV-1-specific AP-1 oligonucleotide 5'-AAACTTGGATGATTCACCTGC-3', position 505–525 in the BPV-1 genome, detected by scanning the BPV-1 genomic sequence with a 7-bp consensus oligonucleotide of AP-1 (5'-TGACTCA-3') using computer program Gap. The oligonucleotides were synthesized in an Applied Biosystems synthesizer using phosphoramitide chemistry and purified further by high performance liquid chromatography. For EMSAs, the annealed oligonucleotides were labeled with [{gamma}-32P]ATP (Amersham Biosciences, 3,000 Ci/mmol) with T4 polynucleotide kinase and gel purified from a 15% polyacrylamide gel. Cellular extracts were prepared according to Schreiber et al. (37) with the only modification that N-N-(L-3-trans-carboxyoxirane-2-carbonyl)-L-leucyl-agmatine (E64) and 4-(2-aminoethyl)-benzolsulfonylfluoride (Pefabloc SC) were included as protease inhibitors in concentrations suggested by the manufacturer (Roche Applied Science). The binding was performed exactly as described (38). The sequence specificity of the binding was controlled in competition experiments by the addition of a 100-fold molar excess of either unlabeled homologous or heterologous oligonucleotides. For monitoring c-Jun/ATF-2 composition in supershift assays, 2 µg of polyclonal antibodies directed against c-Jun or ATF-2 was added, and the reaction was incubated further for 1 h at 4 °C. In detail, the following antibodies (all obtained from Santa Cruz, Biotechnology as TransCRuzTM supershift reagents) were used: c-Jun-Ab, which recognizes both the unphosphorylated and phosphorylated form of c-Jun (epitope corresponding to amino acids 56–69 mapping within the amino-terminal domain of the mouse c-Jun protein); ATF-2 antibody, specific for Thr71-phosphorylated ATF-2). The DNA-protein complexes were resolved on 5.5% non-denaturating polyacrylamide gels (29:1 cross-linking ratio), dried, and exposed overnight to Kodak X-Omat films.

Western Blot Analyses—Total cellular protein extracts were prepared using ice cold RIPA buffer (0.5% deoxycholate, 0.5% Nonidet P-40, 0.5% SDS, 50 mM Tris, pH 7.4, and 100 mM NaCl) supplemented with freshly added protease inhibitor mixture (CompleteTM, Roche Applied Science). The protein concentration was determined by the method of Bradford (39) (Bio-Rad), and 50 µg of total protein was electrophoresed on 10% SDS-polyacrylamide gels under reducing conditions. After electrotransfer to ImmobilonTM-P polyvinylidene difluoride membranes (Millipore Corporation), the membranes were incubated for 1 h at room temperature with blocking solution: TBS (20 mM Tris-HCl, pH 7.6, 0.14 M NaCl) containing 0.1% Tween 20 (Sigma) and 5% skim milk powder (Merck). After blocking, the membranes were incubated with the first antibody (diluted in blocking solution) overnight at 4 °C. The membranes were washed three times with TBS containing 0.1% Tween 20 for 30 min and then incubated for 2 h at room temperature with the second antibody (anti-rabbit or anti-mouse IgG conjugated with horseradish peroxidase) diluted 1:5,000 in blocking solution. Finally the membranes were washed again for 30 min, incubated 2 min with the ECL reagents (Amersham Biosciences), and exposed on Kodak X-Omat films. For stripping, the membranes were incubated with 200 mM NaOH for 5 min and washed with water prior to incubation with an additional antibody. The following polyclonal antibodies were used (all purchased from New England Biolabs): phospho-p38, p38, phospho-JNK, JNK, phospho-ERK1/2, phospho-c-Jun, phospho-ATF-2, and ATF-2. c-Jun antibody, and Cdk2 antibody were from Santa Cruz Biotechnology. The BPV E5 monoclonal antibody was a kind gift from R. Schlegel (Georgetown University, Washington, D. C.). Equal protein transfer and loading were routinely controlled by reincubating the filters with a monoclonal actin-specific antibody (ICN Biomedicals).

p38 MAP Kinase Assay—All steps of the nonradioactive kinase assay system were performed exactly according to the manufacturer's instructions (New England Biolabs). Cells were lysed in buffer containing 20 mM Tris, pH 7.5, 150 mM NaCl, 1 mM EDTA, 1 mM EGTA, 1% Triton, 2.5 mM sodium pyrophosphate, 1 mM-glycerophosphate, 1 mM Na3VO4, and 1 µg/ml leupeptin. The first step includes an immunoprecipitation of p38 MAP kinase from a 100-µg protein extract via immobilized phospho-p38 MAP kinase (Thr180/Tyr182) monoclonal antibody. In vitro kinase assay was performed using purified ATF-2 protein as substrate. ATF-2 phosphorylation was detected by Western blot using phospho-ATF-2 (Thr71) antibody.

Fluorescence-activated Cell Sorter Analysis—For fluorescence analysis, cells were washed twice with phosphate-buffered saline and stained 1 h with 50 µg/ml propidiumiodide + 40 µg/ml RNaseA in phosphate-buffered saline in the dark at 4 °C. Analysis was performed using a BD Biosciences flow cytometer (40). Cell cycle distribution and quantification of flow cytometric data were performed according to Dean and Jett (41). For each measurement, 10,000 cells were counted.

RT-PCR—Total RNA was isolated using the RNeasy kit from Qiagen according to the instructions of the provider. 30 µg of RNA was treated with 1 unit of DNase for 20 min at 37 °C to remove residual genomic DNA. The RT reaction was performed using the Omniscript RT kit from Qiagen; 2 µg of RNA was used for a 20-µl reaction volume to generate cDNA. E2 sequence-specific PCR was performed with 0.5 µl of RT Mix, now containing cDNA, 5 mmol of dNTPs, 5 pmol of primers, and 0.7 unit of Expand High Fidelity Polymerase (Roche Applied Science) in a 20-µl reaction volume using primers for full-length, amino-terminal, and carboxyl-terminal E2 DNA sequences: forward (F) primer, 5'-AGACAGCATGCGAACGTTTA-3'; reverse (R) primer, 5'-TGCTTGGCTCTCTCTTGACA-3'; amino-terminal Rn primer, 5'-TCCTCTTCTTCCTGCCTTGA-3'; carboxyl-terminal Fc primer: 5'-AGCCCAGCCTGTCTCTTCT-3. The PCR program (MJ Research PCR Cycler) was as follows: step 1, denaturation at 95 °C for 1 min; step 2, denaturation at 95 °C for 30 s; step 3, annealing with touch down 65–1 °C/cycle; step 4, elongation at 72 °C for 4 min; step 5, repeat steps 2–4, 19 times; step 6, denaturation at 95 °C for 30 s; step 7, annealing at 55 °C for 30 s; step 8, elongation at 72 °C for 4 min; step 9, repeat steps 6–8, 19 times; step 10, elongation at 72 °C for 12 min and cooling at 4 °C. PCR products were separated on 1% agarose gels and detected after ethidium bromide staining under UV.

Immunoprecipitation and Cdk2 Assay—Cdk2 activity was measured after immunoprecipitation of the protein from cell extracts and phosphorylation of histone H1 as substrate (42). 100 µg of each cell extract (treated and controls) was supplemented with 1 µl of anti-Cdk2 antibody (Santa Cruz) and incubated on ice for 2 h. The following step was the binding of protein-antibody aggregates by A/G-agarose beads and centrifugation to separate the bound complexes from free protein. The beads were washed using lysis buffer (50 mM Tris, 250 mM NaCl, 1% Triton X-100, 5 mM EDTA, 50 mM NaF, 1 mM dithiothreitol, 0,1 mM phenylmethylsulfonyl fluoride, 100 µM natriumvanadate, 1 µg/ml aprotinin, 10 µg/ml soybean trypsin inhibitor, 10 µg/ml tosylphenylalanyl chloromethyl ketone, 5 µg/ml 1-chloro-3-tosylamido-7-amino-2-heptanone) and kinase reaction buffer (50 mM Tris, pH 7.5, 10 mM MgCl2, 1 mM dithiothreitol), and afterward a premix consisting of histone H1 (calf thymus, Calbiochem-Novabiochem), ATP (Roche Applied Science), and radioactive {gamma}-ATP (Amersham Biosciences) was added. The kinase reaction was incubated for 15 min at 30 °C, and the detection of phosphorylated histone H1 was performed after 10% SDS-PAGE, Coomassie staining, and autoradiography of dried gels.


   RESULTS
TOP
 ABSTRACT
 INTRODUCTION
 EXPERIMENTAL PROCEDURES
 RESULTS
DISCUSSION
 REFERENCES
 
AG 555 Selectively Down-regulates BPV-1 Transcription— Because of their structural similarity with tyrosine (Fig. 1, panel A) tyrphostins can block protein-tyrosine kinase activity by binding to the substrate binding site (2). To test the effect of AG 555 on viral transformed cells, BPV-1-transformed mouse fibroblasts (ID13 cells) were treated for different periods of time, and total RNA was examined by Northern blot analysis. As shown in Fig. 1, panel B, cell incubation in the presence of 30 µM AG 555 resulted in a selective down-regulation of the most abundant viral transcripts (27, 43) already 4 h after drug application. To demonstrate that AG 555-mediated BPV-1 suppression was a selective process and not the consequence of a general transcriptional block per se, the RNA filters were rehybridized with endogenous reference genes. Notably, under conditions in which BPV-1 transcription was suppressed, an even costimulatory effect on c-Jun gene expression could be discerned. c-Jun induction was detectable already 2 h after AG 555 addition and remained elevated up to 8–10 h. Subsequent hybridization of the same filters with a housekeeping gene probe ({beta}-actin) demonstrated that suppression was specifically directed against the virus-specific transcription cassette and did not represent the result of a nonspecific transcriptional impairment of the cells by the tyrphostin.



View larger version (43K):
[in this window]
[in a new window]
  		FIG. 1.
Down-regulation of BPV-1 mRNA by AG 555. Panel A, tyrphostin AG 555 structurally resembles tyrosine and erbstatin moieties, but it has additional hydrophobic properties to enhance cell membrane permeability. Panel B, Northern blot analysis. ID13 cells were treated with AG 555 for 2, 4, 6, 8, or 10 h. 5 µg of RNA was separated in a 1% agarose gel. The filters were hybridized with DNA probes encoding BPV-1, c-Jun, and {beta}-actin. Positions of the 28 S and 18 S ribosomal RNA after ethidium bromide staining are indicated. C, untreated cells; D, Me2SO-treated controls; A, treated with 30 µM AG 555.

 

Down-regulation of BPV-1 Transcription and Cell Cycle Arrest: Suppression of Cdk2 Activity—Measuring the cell cycle profile by flow cytometric analysis under conditions in which BPV-1 expression was found to be down-regulated, the majority of ID13 cells were growth-arrested with an accumulation of the cells at the late S/early G2 boundary, whereas the G1 phase was diminished (Fig. 2, panel A). For example, considering the fluorescence-activated cell sorter profile 8 h after AG 555 treatment, an increase of the S/G2 phase from 7.7 to 18.5% and from 12 to 25% and a decrease of G1 from 75 to 43%, respectively, could be noted (see Fig. 2, panel A). To analyze whether the inhibition of BPV-1 transcription and cell cycle arrest correlated with cyclin-dependent kinase activity suppression, cyclin-Cdk2 complexes were first immunoprecipitated with a Cdk2-specific antibody and subsequently functionally tested in an in vitro phosphorylation assay using histone H1 as substrate (Fig. 2, panel B, upper part). Compared with the untreated controls, Cdk2 remained active up to 2 h but declined significantly between 6 and 8 h after the addition of AG 555.



View larger version (37K):
[in this window]
[in a new window]
  		FIG. 2.
Effect of AG 555 on cell cycle distribution and Cdk activity. Panel A, flow cytometric analysis of ID13 cells 8 h after treatment with 30 µM AG 555. The percentages of cells within the different cell cycle phases (G1, S, G2) are indicated (ordinate, number of cells; abscissa, relative fluorescence intensity). 1–4 indicate the sub-G1, G1, S, and G2 peaks, respectively. Panel B, the upper part shows Coomassie staining of the gel to demonstrate equal input of H1 to the kinase assay. The lower part is autoradiography. Cdk2 complexes were immunoprecipitated and assayed for their activity in phosphorylating histone H1 as substrate. Panel C, Western blot analysis of Cdk2 expression. 50 µg of total cellular extracts was separated in a 10% SDS-polyacrylamide gel and immunoblotted with a specific antibody directed against Cdk2. Equal loading was verified by incubation with an actin antibody. C, untreated cells; D, Me2SO-treated controls; A, treated with AG 555. Panel D, Western analysis of E5 oncoprotein expression. 50 µg of total cellular extracts was separated in a 15% SDS-polyacrylamide gel. The filters were incubated with specific antibodies against BPV-1 E5, Ha-ras, and actin, respectively.

 

To exclude that Cdk2 activity was reduced because of quantitative changes in Cdk2 itself, total cellular extracts were monitored by Western blot analysis. Consecutive incubation of the filter with specific antibodies against Cdk2 and actin as internal loading control confirmed equal Cdk2 expression (Fig. 2, panel C). In addition, consistent with the transcriptional data presented above (Fig. 1, panel B), the level of the E5 oncoprotein was down-regulated in the same time range, whereas the expression of Ha-ras and actin as internal reference was not affected (Fig. 2, panel D). These results suggest that AG 555 was efficiently inducing cell cycle arrest by negatively interfering with BPV-1 transcription and Cdk2 function.

MAP Kinase Pathway Activation by AG 555—Because c-Jun expression was induced upon AG 555 treatment, we reasoned that tyrphostin treatment may act as a cellular stress signal (for review, see Ref. 44) that activates the MAP kinase pathway and in turn downstream target proteins. Mammalian MAP kinases consist of three groups: ERK, JNK, and the p38 MAP kinases (45). To prove whether AG 555 was affecting MAP kinase activity, Western blot analyses using phosphorylation-specific antibodies raised against ERK, JNK, and p38 were performed. Fig. 3, panel A, shows that only the stress kinases JNK and p38 were phosphorylated, reaching a maximum between 4 and 6 h after the addition of AG 555. In contrast, ERK1 and ERK2 were unaltered under the same experimental conditions. Phosphorylation could be not attributed to an enhanced protein synthesis because control incubations of the filters with nonphosphorylation-specific antibodies revealed that the net amount of the corresponding proteins was the same.



View larger version (31K):
[in this window]
[in a new window]
  		FIG. 3.
AG 555 activates the MAP kinase pathway. Panel A, Western blot analysis of p38, JNK, and ERK1/2 MAP kinases. 50 µg of total cellular extract/lane was separated in three identical 10% SDS-polyacrylamide gels. After transfer, the filters were either incubated with phosphorylation-specific (indicated as P-p38, P-JNK, and P-ERK1/2, respectively) or phosphorylation-unspecific antibodies. The molecular masses are indicated in kDa (see arrowheads). Panel B, Western blot of c-Jun and phospho-Jun. Equal loading and protein transfer were confirmed by incubating one filter with an actin-specific antibody (actin). Panel C, nonradioactive kinase assay to monitor p38 activity. Upper part, Western blot of p38 (total Triton X-100 extract) demonstrating the time course of phosphorylated p38 MAP kinase accumulation after AG 555 treatment; equal loading was verified by incubation with an actin antibody. Lower part, detection of increased phosphorylated ATF-2 after incubation of equal amounts of purified ATF-2 together with the immunoprecipitated p38 MAP kinase. C, untreated cells; D, Me2SO-treated controls; A, treated with 30 µM AG 555.

 

p38 MAP kinases are normally activated by dual phosphorylation on Thr and Tyr within a Thr-Gly-Tyr motif (46). It was therefore unexpected that a tyrphostin, which can potentially interfere with tyrosine phosphorylation (2), can activate p38. Because the p38 antibody used cannot distinguish between these two phosphorylation sites, it was mandatory to test whether phosphorylation was in fact accompanied with an increased enzymatic activity. p38 was therefore first immunoprecipitated from nuclear extracts and subsequently assayed in vitro using purified ATF-2 (in the presence of ATP) as a substrate. Phosphorylation of ATF-2 was detectable already 30 min after the addition of AG 555, which coincides temporarily with p38 activation (Fig. 3, panel B) but precedes viral suppression (see below). JNK activity was measured in vivo by probing nuclear extracts with c-Jun phosphorylation-specific antibodies directed against the serine residues at positions 63 and 73 within the amino-terminal transactivating domain. As depicted in Fig. 3, panel B, even though c-Jun was induced on a transcriptional level (Fig. 1, panel B), no enhanced accumulation of the corresponding protein could be noted. These data indicate that the biological outcome of AG 555-mediated MAP kinase activation was restricted mainly to post-translational phosphorylation events on c-Jun and ATF-2.

Identification of a Potential Intragenic AP-1 site within the BPV-1 Genome—To determine whether the repression of viral transcription is linked causally with MAP kinase activation, we anticipated that the activation of the AP-1 family members c-Jun and ATF-2 may either directly or indirectly influence BPV-1 expression. Because no AP-1 binding site within the BPV-1 genome has been described until now, we scanned the nucleotide sequence for putative binding sites with the computer program Gap using the 12-O-tetradecanoylphorbol-13-acetate-responsive sequence 5'-TGA(G/C)TCA-3' (TRE) as search criterion. Several potential sites were found, whereby only the intragenic AP-1 sequence (referred to as BAP-1 for BPV AP-1 site 2, nucleotide positions 505–525, 5'-TGATTCA-3') revealed binding in EMSAs using nuclear extracts derived from ID13 cells (Fig. 4, panel A). Specificity was confirmed by homologous competition with BAP-1 or by addition of a 100-fold molar excess of unlabeled AP-1 oligonucleotides harboring either the consensus sequence derived from the collagenase promoter or from the TRE sequence. Binding, however, cannot be abrogated after competition with a heterologous SP-1 oligonucleotide.



View larger version (51K):
[in this window]
[in a new window]
  		FIG. 4.
Detection of an AP-1 binding element in the BPV-1 genome. Panel A, the left part demonstrates binding selectivity at the BAP-1 sequence. Competition can be achieved by addition of 100-fold molar amounts of unlabeled BAP-1, AP-1, and TRE oligonucleotides, but not with oligonucleotides harboring a SP1 recognition site. The right part shows that BAP-1 can also compete binding to labeled AP-1 consensus oligonucleotides. Panel B, EMSA of BAP-1 binding after AG 555 incubation for different periods of time. Panel C, supershift EMSA after the addition of AG 555 using antibodies against c-Jun and phosphorylated ATF-2 (P-ATF-2). Panel D, linear map of the BPV-1 genome. The localization of the different promoters (P7185, late promoter; P7949, P1; P89, P2; P890, P3; P2443, P4; P3080, P5)) relative to the ORFs (E, early; L, late) are indicated. URR, upstream regulatory region.

 

Having verified the authenticity of the novel AP-1 binding site within the BPV-1 genome (Fig. 4, panel A), it was of interest to monitor quantitative and qualitative changes after AG 555 treatment. Notably, EMSAs completely failed to detect any increased AP-1 binding affinity using 32P-labeled BAP-1 oligonucleotides as probe (Fig. 4, panel B). Application of a c-Jun antibody in the binding reaction (supershift) demonstrated that c-Jun was only slightly elevated within the AP-1 complex, whereas the amount of phosphorylated ATF-2, which normally binds to the ATF/cAMP-responsive binding protein consensus sequence 5'-TG/TACGTCA-3' (47), became significantly enhanced (Fig. 4, panel C). Elevated association and dimerization of ATF-2 with c-Jun seem to be specific because other AP-1 family members such as c-Fos or Fra-1 were not increased (data not shown).

In the next set of experiments we asked whether MAP kinase and in particular p38 activation was a prerequisite for the negative regulatory effect on viral gene expression. It is known that c-Jun transcription becomes enhanced through an autoregulatory mechanism, which is mediated via binding of c-Jun/ATF-2 heterodimers to its own promoter sequence (34). If there was a divergent regulation on BPV-1 and c-Jun expression, one should expect that in the same way as the transcriptional block on BPV-1 is relieved, the c-Jun steady-state level should be reduced. To answer this question, ID13 cells were treated with AG 555 together with SB 203580, an inhibitor of p38 MAP kinase activity (48). Northern blot analysis revealed that this was indeed the case (Fig. 5). Simultaneous incubation with AG 555 and SB 203580 led to significant re-expression of BPV-1, whereas the c-Jun-specific signal was diminished. These results strongly suggest that p38 activation and phosphorylation of its downstream target ATF-2 play a crucial role in tyrphostin-mediated BPV-1 repression.



View larger version (52K):
[in this window]
[in a new window]
  		FIG. 5.
Blockage of the diverse BPV-1/c-Jun transcriptional regulation after AG 555 by simultaneous treatment with the p38 MAP kinase inhibitor SB 203580. For Northern blot analysis ID13 cells were treated either with AG 555 (A)/SB 203580 (SB) alone or together (SB/A) for 7 h. 5 µg of RNA was separated in a 1% agarose gel. The filters were hybridized with DNA probes encoding BPV-1, c-Jun, and {beta}-actin. Positions of the 28 S and 18 S ribosomal RNA after ethidium bromide staining are indicated. C, untreated cells; D, Me2SO-treated controls. The filter was hybridized with BPV-1-, c-Jun-, and {beta}-actin-specific probes.

 

The Viral Transcriptional Transactivator E2 is Down-regulated, whereas the Level of Short E2 Encoding the Repressor Form Remained Constant during AG 555 Treatment—Although the functional role of BAP-1 is not yet clear, we reasoned that c-Jun/ATF-2 binding could affect BPV-1 expression by perturbing viral transcription initiated at different promoters located both in the upstream regulatory region and within the early coding region (for schematic overview, see Fig. 4, panel D). A well characterized mechanism that inherently interferes negatively with transcription is mediated by the viral E2 protein itself (49, 50). Depending on which promoter is used, two forms of E2 can by synthesized from differently spliced mRNA species: a transactivator, starting from position P2443 (Fig. 4, panel D), consists of the full-length protein harboring an amino-terminal activator domain as well as a carboxyl-terminal DNA and dimerization region (51). Alternatively, there also exist two truncated forms of E2, initiating from position P890 and P3080 (Fig. 4, panel D) which lack the transactivation domain and can therefore act as transcriptional repressors (52). To determine whether treatment of AG 555 had an effect on the ratio between the different transcripts encoding either the repressor (E2-TR) or activator form of E2 (E2-TA), RT-PCR analyses were performed (Fig. 6). Using selected primers diagnostic for the repressor (the smaller carboxyl-terminal part, referred as Fc-R, see Fig. 6, lower panel), a 303-bp PCR product was accumulated whose amount was not quantitatively changed. In contrast, trapping transcripts encoding the complete transactivator (referred as F-Rn, indicative for the amino terminus and therefore encoding the entire E2), the 220-bp PCR product was drastically diminished upon AG 555 treatment. The usage of the cellular glyceraldehyde-3-phosphate dehydrogenase gene as internal control confirmed the selectivity of this process. Because the transactivator function is required to stimulate transcription within the viral promoters (53), E2-TA depletion in favor to E2-TR apparently accounts for the suppressive effect after tyrphostin application.



View larger version (30K):
[in this window]
[in a new window]
  		FIG. 6.
Selective suppression of E2 transactivator and concomitant maintenance of E2 repressor transcription after AG 555 treatment. Panel A, RT-PCR analysis. Top part, glyceraldehyde-3-phosphate dehydrogenase (GAPDH); middle part, PCR product (303 bp) encompassing the carboxyl-terminal ORF of E2 (repressor); bottom part, PCR product (220 bp) trapping the amino-terminal part of the E2 ORF (transactivator). Panel B, schematic overview of the E2 ORF. The derivation of the primers used for PCR analysis and the size of the expected fragments are indicated.

 


   DISCUSSION
TOP
 ABSTRACT
 INTRODUCTION
 EXPERIMENTAL PROCEDURES
 RESULTS
 DISCUSSION
REFERENCES
 
Tyrphostins are useful tools for negatively interfering with enhanced tyrosine phosphorylation in many malignant disorders (2). Some tyrphostins were shown to possess strong anti-proliferative activity without having identified the exact target. Using BPV-1-transformed C127 mouse fibroblasts (ID13 cells) as the model system, we studied the effect of the tyrphostin AG 555 in the context of virus-induced carcinogenesis. Treatment of ID13 cells with 30 µM AG 555 for different periods of time resulted in a selective down-regulation of viral transcription (Fig. 1, panel B). However, the mRNA decline followed a different kinetic compared with actinomycin D, known to block RNA polymerase transcription nonspecifically by intercalating into the DNA (data not shown). The slight initial increase and the subsequent drop of the viral transcripts either argued for delayed regulatory pathway acting at the level of initiation of transcription or for a post-transcriptional control mechanism. Although the steady-state level of BPV-1 mRNA can be enhanced by cycloheximide (54), short term blockage of protein synthesis for 1 h was not abrogating the suppressive effect on viral transcription after a 7-h AG 555 treatment (data not shown). This favored the assumption that AG 555 apparently induced an alternative mode of transcriptional control rather than through post-transcriptional labilization of the BPV-1-specific RNAs (see below).

As further demonstrated, down-regulation of viral transcription temporarily correlated with growth arrest and cyclin-dependent kinase suppression (Fig. 2, panels A and B). However, it should be stressed that this coincidence may not necessarily be the consequence of the reduction of the major viral oncoprotein E5 (Fig. 2, panel D) because the same situation can be found when the nontransformed, but still immortalized, C127 mouse fibroblasts were monitored (data not shown). On the other hand, it seems that whenever there is enhanced tyrosine phosphorylation to threshold levels, tyrphostins have growth-inhibitory properties (55). Consistent with this notion is that AG 555 is capable of blocking cell proliferation of HPV-16-immortalized human keratinocytes (56, 57) and psoriatic keratinocytes, where persistent autocrine/paracrine stimulation of the EGF receptors by transforming growth factor-{alpha} can be discerned (58).

The expression of immediate-early genes such as c-Jun, found to be activated upon AG 555 addition (Fig. 1, panel B), is tightly controlled by the MAP kinase pathway (for review, see Ref. 44). We therefore anticipated that tyrphostin treatment may act as stress signal, similar to the situation described recently in human platelets treated using genistein as a tyrosine kinase inhibitor (59). As depicted in Fig. 3, panel A, AG 555 selectively induced JNK and p38 phosphorylation, whereas ERK1/2 MAP kinase was not affected. Enhanced c-Jun expression can be explained by phosphorylation of pre-existing c-Jun and ATF-2 proteins (Fig. 3, panels B and C), which in turn stimulate transcription through binding of c-Jun/ATF-2 dimers to related cis-regulatory sequences within the c-Jun promoter (for review, see Ref. 60).

EMSAs revealed that c-Jun became dimerized with increased levels of phosphorylated ATF-2, which bind to a novel identified intragenic AP-1 sequence motif (BAP-1) within the E7 ORF (Fig. 4, panels A and C). Notably, even though c-Jun mRNA was increased, the net amount of DNA binding at the BAP-1 sequence was not affected (Fig. 4, panel B). In contrast to "high risk" HPVs, where the transcription factor AP-1 and its composition are apparently part of an intracellular surveillance mechanism regulating both E6/E7 transcription and tumorigenicity (38, 61, 62), a similar role for AP-1 and its corresponding binding site has not yet been described for BPV-1. Although it is currently not clear how this binding site affects the usage of BPV-1 upstream and downstream localized promoters in the whole genomic framework (see the schematic overview in Fig. 4, panel D), divergent transcriptional regulation of c-Jun and BPV-1 gene expression became drastically abrogated by blocking p38 activity with SB 203580 (63) (Fig. 5). The explanation of why no complete reversion to initial steady-state levels could be accomplished is probably due to the redundancy of the MAP kinase network as both JNK and p38 can phosphorylate c-Jun and ATF-2 (44). It is reasonable to assume that phospho-ATF-2 may negatively influence BPV-1 expression. Although ATF-2 is generally considered as a positive regulator (34), the involvement of ATF-2 in gene repression is not without a precedent. Notably, as shown for hepatitis B virus, ATF-2 can down-regulate hepatitis B virus X promoter activity by competing for the AP-1 binding site through enhanced Jun/ATF-2 heterodimer formation (64). How this is exactly mediated in the case of BPV-1 remains to be elucidated.

Considering the small size, the existence of at least five as yet characterized promoters and the circularity of DNA (a circular permutated viral template), BPV-1 can be regarded as an episomal enhanceosome, where the occupancy of the novel intragenic cis-regulatory element at position 505–525 by phosphorylated Jun/ATF-2 can also affect other promoters, in particular promoters controlling the transcription of the E2 protein (see Fig. 4, panel D). E2 seems to be the master regulator protein controlling not only the viral copy number (65) but also the transcriptional fine tuning by utilizing different promoters (28). The E2 protein can be synthesized from differently spliced mRNA species found in both transformed cells and differentiating cells. When started from the promoter at position P2443 (Fig. 4, panel D), a full-length transactivator protein is generated, harboring an amino-terminal activator domain as well as a carboxyl-terminal DNA and dimerization region (51). On the other hand, there also exist two shortened forms of E2, initiating from positions P890 and P3080, respectively (Fig. 4, panel D). The E8/E2 as well as the E2-TR gene products lack the transactivation domain and can therefore act as transcriptional repressors (52). In the context of the entire genome, however, dysfunction of the E8/E2 protein has little effect on viral gene expression, whereas disruption of the E2 repressor E2-TR resulted in an increase of the transformation potential (50).

DNase I footprinting analyses have revealed that there are 17 different E2 binding sites within the BPV-1 genome, which differ in their affinities and equilibrium constants (66). In addition to the E2 binding sites within the upstream regulatory region, there are also recognition positions for E2 immediately upstream of the P2443 and the P3080 promoter (67). The former, which is controlled by an E2 autoregulatory loop (68), is responsible for the synthesis of the most abundant mRNA encoding the transforming protein E5 (27). AG 555 is apparently triggering a cascade of distinct regulatory steps, which resulted in a disturbance of the ratio between E2-specific RNAs encoding either the transactivator (E2-TA) or the transrepressor function (E2-TR) of E2 (Fig. 6). Because the P2–P5 promoters (Fig. 4, panel D) are all stimulated by the E2 transactivator function (28), the selective reduction of E2-TA in favor of E2-TR probably accounts for the ultimate suppression of viral transcription. These findings indicate that tyrosine kinase signaling obviously plays an important role in the maintenance of the BPV-1 transforming activity.

Are these results transferable to human papillomaviruses? With the exception of the HPV-16-positive W12 cells (69) or the HPV-31-containing CIN612 cells (70), not many human keratinocyte lines harbor stable episomes. In most cervical carcinoma cells, HPV is found to be integrated where the balanced modulation of early gene expression via the antagonistic action of E2 is destroyed (for review, see Ref. 21). However, with respect to the distribution of additional regulatory elements upstream from and within the E2 ORF (71, 72), it would be interesting to test AG 555 and the role of E2 on cell lines carrying HPV in an episomal state.


   FOOTNOTES
 
* This work was supported by the Cooperation Program in Cancer Research of the Deutsches Krebsforschungszentrum and the Israeli Ministry of Science. The costs of publication of this article were defrayed in part by the payment of page charges. This article must therefore be hereby marked "advertisement" in accordance with 18 U.S.C. Section 1734 solely to indicate this fact. Back

To whom correspondence should be addressed: Abteilung Virale Transformationsmechanismen, Deutsches Krebsforschungszentrum, Forschungsschwerpunkt Angewandte Tumorvirologie, Im Neuenheimer Feld 242, Heidelberg 69120, Germany. Tel.: 49-6221-42-4900; Fax: 49-6221-42-4902; E-mail: f.roesl{at}dkfz.de.

1 The abbreviations used are: EGF, epidermal growth factor; ATF-2, activating transcription factor 2; BPV-1, bovine papillomavirus type 1; EMSA, electrophoretic mobility shift assay; ERK, extracellular signal-regulated kinase; HPV, human papillomavirus; IGF, insulin-like growth factor; JNK, c-Jun NH2-terminal kinase; MAP, mitogen-activated protein; Me2SO, dimethyl sulfoxide; ORF, open reading frame; RT, reverse transcription. Back


   ACKNOWLEDGMENTS
 
We thank K.-J. Hutter and U. Soto for help with the flow cytometric analysis and EMSAs, H. zur Hausen for continuous support, and Julia Nafz for reading the manuscript.



   REFERENCES
TOP
 ABSTRACT
 INTRODUCTION
 EXPERIMENTAL PROCEDURES
 RESULTS
 DISCUSSION
 REFERENCES
 

  1. Ullrich, A., and Schlessinger, J. (1990) Cell 61, 203–212[CrossRef][Medline] [Order article via Infotrieve]
  2. Levitzki, A. (1999) Pharmacol. Ther. 82, 231–239[CrossRef][Medline] [Order article via Infotrieve]
  3. Levitzki, A., and Gazit, A. (1995) Science 267, 1782–1788[Abstract/Free Full Text]
  4. Lipson, K. E., Pang, L., Huber, L. J., Chen, H., Tsai, J. M., Hirth, P., Gazit, A., Levitzki, A., and McMahon, G. (1998) J. Pharmacol. Exp. Ther. 285, 844–852[Abstract/Free Full Text]
  5. Ben-Bassat, H., Vardi, D. V., Gazit, A., Klaus, S. N., Chaouat, M., Hartzstark, Z., and Levitzki, A. (1995) Exp. Dermatol. 4, 82–88[CrossRef][Medline] [Order article via Infotrieve]
  6. Brenner, T., Poradosu, E., Soffer, D., Sicsic, C., Gazit, A., and Levitzki, A. (1998) Exp. Neurol. 154, 489–498[CrossRef][Medline] [Order article via Infotrieve]
  7. Maruo, T., Yamasaki, M., Ladines-Llave, C. A., and Mochizuki, M. (1992) Cancer 69, 1182–1187[Medline] [Order article via Infotrieve]
  8. Morrione, A., DeAngelis, T., and Baserga, R. (1995) J. Virol. 69, 5300–5303[Abstract]
  9. Crusius, K., Auvinen, E., and Alonso, A. (1997) Oncogene 15, 1437–1444[CrossRef][Medline] [Order article via Infotrieve]
  10. Petti, L., and DiMaio, D. (1992) Proc. Natl. Acad. Sci. U. S. A. 89, 6736–6740[Abstract/Free Full Text]
  11. Klein, O., Kegler-Ebo, D., Su, J., Smith, S., and DiMaio, D. (1999) J. Virol. 73, 3264–3272[Abstract/Free Full Text]
  12. Martin, P., Vass, W. C., Schiller, J. T., Lowy, D. R., and Velu, T. J. (1989) Cell 59, 21–32[CrossRef][Medline] [Order article via Infotrieve]
  13. Leechanachai, P., Banks, L., Moreau, F., and Matlashewski, G. (1992) Oncogene 7, 19–25[Medline] [Order article via Infotrieve]
  14. Jeon, S., Allen-Hoffmann, B. L., and Lambert, P. F. (1995) J. Virol. 69, 2989–2997[Abstract]
  15. Kabsch, K., and Alonso, A. (2002) J. Virol. 76, 12162–12172[Abstract/Free Full Text]
  16. Alazawi, W., Pett, M., Arch, B., Scott, L., Freeman, T., Stanley, M. A., and Colem, N. (2002) Cancer Res. 62, 6959–6965[Abstract/Free Full Text]
  17. Nakamura, K., Hongo, A., Kodama, J., Miyagi, Y., Yoshinouchi, M., and Kudo, T. (2000) Cancer Res. 60, 760–765[Abstract/Free Full Text]
  18. Mathur, S. P., Mathur, R. S., Rust, P. F., and Young, R. C. (2000) Am. J. Reprod. Immunol. 46, 280–287
  19. Law, M. F., Lowy, D. R., Dvoretzky, I., and Howley, P. M. (1981) Proc. Natl. Acad. Sci. U. S. A. 78, 2727–2731[Abstract/Free Full Text]
  20. DiMaio, D., Guralski, D., and Schiller, J. T. (1986) Proc. Natl. Acad. Sci. U. S. A. 83, 1797–1801[Abstract/Free Full Text]
  21. zur Hausen, H. (2002) Nature Rev. Cancer 5, 342–350
  22. Rabson, M. S., Yee, C., Yang, Y. C., and Howley, P. M. (1986) J. Virol. 60, 626–634[Abstract/Free Full Text]
  23. Tong, X., and Howley, P. M. (1997) Proc. Natl. Acad. Sci. U. S. A. 94, 4412–4417[Abstract/Free Full Text]
  24. Dürst, M., Kleinheinz, A., Hotz, M., and Gissmann, L. (1985) J. Gen. Virol. 66, 1515–1522[Abstract/Free Full Text]
  25. Rösl, F., Waldeck, W., Zentgraf, H., and Sauer, G. (1986) J. Virol. 58, 500–507[Abstract/Free Full Text]
  26. Rösl, F., and Waldeck, W. (1991) Mol. Carcinogenesis 4, 248–256
  27. Baker, C. C., and Howley, P. M. (1987) EMBO J. 6, 1027–1035[Medline] [Order article via Infotrieve]
  28. Szymanski, P., and Stenlund, A. (1991) J. Virol. 65, 5710–5720[Abstract/Free Full Text]
  29. Jeon, S., and Lambert, P. F. (1995) Proc. Natl. Acad. Sci. U. S. A. 92, 1654–1658[Abstract/Free Full Text]
  30. Chomczynski, P., and Sacchi, N. (1987) Anal. Biochem. 162, 156–159[Medline] [Order article via Infotrieve]
  31. Khandjian, E. W., and Meric, C. (1986) Anal. Biochem. 159, 227–232[CrossRef][Medline] [Order article via Infotrieve]
  32. Feinberg, A. P., and Vogelstein, B. (1983) Anal. Biol. 132, 6–13
  33. Chen, E. Y., Howley, P. M., Levinson, A. D., and Seeburg, P. H. (1982) Nature 299, 529–534[CrossRef][Medline] [Order article via Infotrieve]
  34. Angel, P., and Karin, M. (1991) Biochim. Biophys. Acta 1072, 129–157[Medline] [Order article via Infotrieve]
  35. Gunning, P., Ponte, P., Okayama, H., Engel, J., Blau, H., and Kedes, L. (1983) Mol. Cell. Biol. 3, 787–795[Abstract/Free Full Text]
  36. Dynan, W. S, and Tjian, R. (1983) Cell 35, 79–87[CrossRef][Medline] [Order article via Infotrieve]
  37. Schreiber, E., Matthias, P., Muller, M. M., and Schaffner, W. (1989) Nucleic Acids Res. 17, 6419[Free Full Text]
  38. Soto, U., Das, B. C., Lengert, M., Finzer, P., zur Hausen, H., and Rösl, F. (1999) Oncogene 18, 3187–3198[CrossRef][Medline] [Order article via Infotrieve]
  39. Bradford, M. M. (1976) Anal. Biochem. 72, 248–254[CrossRef][Medline] [Order article via Infotrieve]
  40. Larsen, J. K., Munch-Petersen, B., Christiansen, J., and Jorgensen, K. (1986) Cytometry 1, 54–63
  41. Dean, P. N., and Jett, J. H. (1974) J. Cell Biol. 60, 523–527[Free Full Text]
  42. Blomberg, I., and Hoffmann, I. (1999) Mol. Cell. Biol. 19, 6183–6194[Abstract/Free Full Text]
  43. Barksdale, S. K., and Baker, C. C. (1993) J. Virol. 67, 5605–5616[Abstract/Free Full Text]
  44. Ichijo, H. (1999) Oncogene 18, 6087–6093[CrossRef][Medline] [Order article via Infotrieve]
  45. Schaeffer, J. J., and Weber, M. J. (1999) Mol. Cell. Biol. 19, 2435–2444[Free Full Text]
  46. Raingeaud, J., Gupta, S., Rogers, J. S., Dickens, M., Han, J., Ulevitch, R. J., and Davis, R. J. (1995) J. Biol. Chem. 270, 7420–7426[Abstract/Free Full Text]
  47. Hai, T., and Curran, T. (1991) Proc. Natl. Acad. Sci. U. S. A. 88, 3720–3724[Abstract/Free Full Text]
  48. Eyers, P. A., van den Ijssel, P., Quinlan, R. A., Goedert, M., and Cohen P. (1999) FEBS Lett. 451, 191–196[CrossRef][Medline] [Order article via Infotrieve]
  49. Hubbert, N. L., Schiller, J. T., Lowy, D. R., and Androphy, E. J. (1988) Proc. Natl. Acad. Sci. U. S. A. 85, 5864–5868[Abstract/Free Full Text]
  50. Lambert, P. F., Monk, B. C., and Howley, P. M. (1990) J. Virol. 64, 950–956[Abstract/Free Full Text]
  51. Spalholz, B. A., Yang, Y. C., and Howley, P. M. (1985) Cell 42, 183–191[CrossRef][Medline] [Order article via Infotrieve]
  52. Choe, J., Vaillancourt, P., Stenlund, A., and Botchan, M. (1989) J. Virol. 63, 1743–1755[Abstract/Free Full Text]
  53. Abroi, A., Kurg, R., and Ustav, M. (1996) J. Virol. 70, 6169–6179[Abstract]
  54. Kleiner, E., Dietrich, W., and Pfister, H. (1986) EMBO J. 5, 1945–1950[Medline] [Order article via Infotrieve]
  55. Kleinberger-Doron, N., Shelah, N., Capone, R., Gazit, A., and Levitzki, A. (1998) Exp. Cell Res. 241, 340–351[CrossRef][Medline] [Order article via Infotrieve]
  56. Ben-Bassat, H., Rosenbaum-Mitrani, S., Hartzstark, Z., Shlomai, Z., Kleinberger-Doron, N., Gazit, A., Plowman, G., Levitzki, R., Tsvieli, R., and Levitzki, A. (1997) Cancer Res. 57, 3741–3750[Abstract/Free Full Text]
  57. Ben-Bassat, H., Rosenbaum-Mitrani, S., Hartzstark, Z., Levitzki, R., Chaouat, M., Shlomai, Z., Klein, B. Y., Kleinberger-Doron, N., Gazit, A., Tsvieli, R., and Levitzki, A. (1999) J. Pharmacol. Exp. Ther. 290, 1442–1457[Abstract/Free Full Text]
  58. Powell, T. J., Ben-Bassat, H., Klein, B. Y., Chen, H., Shenoy, N., McCollough, J., Narog, B., Gazit, A., Harzstark, Z., Chaouat, M., Levitzki, R., Tang, C., McMahon, J., Shawver, L., and Levitzki, A. (1999) Br. J. Dermatol. 141, 802–810[CrossRef][Medline] [Order article via Infotrieve]
  59. Kansra, S. V., Reddy, M. A., Weng, Y., and Shukla, S. D. (1999) Pharmacol. Res. 39, 21–31[CrossRef][Medline] [Order article via Infotrieve]
  60. Karin, M., Liu, Z., and Zandi, E. (1997) Curr. Opin. Cell Biol. 9, 240–246[CrossRef][Medline] [Order article via Infotrieve]
  61. Soto, U., Denk, C., Finzer, P., Hutter, K. J., zur Hausen, H., and Rösl, F. (2000) Int. J. Cancer 86, 811–817[CrossRef][Medline] [Order article via Infotrieve]
  62. Talora, C., Sgroi, D. C., Crum, C. P., and Dotto, G. P. (2002) Genes Dev. 16, 2252–2263[Abstract/Free Full Text]
  63. Enslen, H., Raingeaud, J., and Davis, R. J. (1998) J. Biol. Chem. 273, 1741–1748[Abstract/Free Full Text]
  64. Choi, C. Y., Choi, B. H., Park, G. T., and Rho, H. M. (1997) J. Biol. Chem. 272, 16934–16939[Abstract/Free Full Text]
  65. Winokur, P. L., and McBride, A. A. (1992) EMBO J. 11, 4111–4118[Medline] [Order article via Infotrieve]
  66. Li, R., Knight, J., Bream, G., Stenlund, A., and Botchan, M. (1989) Genes Dev. 3, 510–526[Abstract/Free Full Text]
  67. Spalholz, B. A., Vande Pol, S. B., and Howley, P. M. (1991) J. Virol. 65, 743–753[Abstract/Free Full Text]
  68. Hermonat, P. L., Spalholz, B. A., and Howley, P. M. (1988) EMBO J. 7, 2815–2822[Medline] [Order article via Infotrieve]
  69. Stanley, M. A., Browne, H. M., Appleby, M., and Minson, A. C. (1989) Int. J. Cancer 43, 672–676[Medline] [Order article via Infotrieve]
  70. Hummel, M., Hudson, J. B., and Laimins, L. A. (1992) J. Virol. 66, 6070–6080[Abstract/Free Full Text]
  71. Karlen, S., and Beard, P. (1993) J. Virol. 67, 4296–4306[Abstract/Free Full Text]
  72. Kim, K. Y., and Taylor, M. W. (2003) J. Med. Virol. 69, 122–131[CrossRef][Medline] [Order article via Infotrieve]

Add to CiteULike CiteULike   Add to Complore Complore   Add to Connotea Connotea   Add to Del.icio.us Del.icio.us   Add to Digg Digg   Add to Reddit Reddit   Add to Technorati Technorati    What's this?



This Article
Right arrow Abstract Freely available
Right arrow Full Text (PDF)
Right arrow All Versions of this Article:
278/39/37306    most recent
M304449200v1
Right arrow Submit a Letter to Editor
Right arrow Alert me when this article is cited
Right arrow Alert me when eLetters are posted
Right arrow Alert me if a correction is posted
Right arrow Citation Map
Services
Right arrow Email this article to a friend
Right arrow Similar articles in this journal
Right arrow Similar articles in PubMed
Right arrow Alert me to new issues of the journal
Right arrow Download to citation manager
Right arrowRequest Permissions
Citing Articles
Right arrow Citing Articles via Google Scholar
Google Scholar
Right arrow Articles by Baars, S.
Right arrow Articles by Rösl, F.
Right arrow Search for Related Content
PubMed
Right arrow PubMed Citation
Right arrow Articles by Baars, S.
Right arrow Articles by Rösl, F.
Social Bookmarking
Add to CiteULike   Add to Complore   Add to Connotea   Add to Del.icio.us   Add to Digg   Add to Reddit   Add to Technorati  
What's this?

HOME HELP FEEDBACK SUBSCRIPTIONS ARCHIVE SEARCH TABLE OF CONTENTS
 All ASBMB Journals   Molecular and Cellular Proteomics 
 Journal of Lipid Research   ASBMB Today 
Copyright © 2003 by the American Society for Biochemistry and Molecular Biology.
Advertisement
spacer
Advertisement
Advertisement