Replication interference between human papillomavirus types 16 and 18 mediated by heterologous E1 helicases
Virology Journalvolume 11, Article number: 11 (2014)
Co-infection of multiple genotypes of human papillomavirus (HPV) is commonly observed among women with abnormal cervical cytology, but how different HPVs interact with each other in the same cell is not clearly understood. A previous study using cultured keratinocytes revealed that genome replication of one HPV type is inhibited by co-existence of the genome of another HPV type, suggesting that replication interference occurs between different HPV types when co-infected; however, molecular mechanisms underlying inter-type replication interference have not been fully explored.
Replication interference between two most prevalent HPV types, HPV16 and HPV18, was examined in HPV-negative C33A cervical carcinoma cells co-transfected with genomes of HPV16 and HPV18 together with expression plasmids for E1/E2 of both types. Levels of HPV16/18 genome replication were measured by quantitative real-time PCR. Physical interaction between HPV16/18 E1s was assessed by co-immunoprecipitation assays in the cell lysates.
The replication of HPV16 and HPV18 genomes was suppressed by co-expression of E1/E2 of heterologous types. The interference was mediated by the heterologous E1, but not E2. The oligomerization domain of HPV16 E1 was essential for HPV18 replication inhibition, whereas the helicase domain was dispensable. HPV16 E1 co-precipitated with HPV18 E1 in the cell lysates, and an HPV16 E1 mutant Y379A, which bound to HPV18 E1 less efficiently, failed to inhibit HPV18 replication.
Co-infection of a single cell with both HPV16 and HPV18 results in replication interference between them, and physical interaction between the heterologous E1s is responsible for the interference. Heterooligomers composed of HPV16/18 E1s may lack the ability to support HPV genome replication.
Human papillomavirus (HPV) has a circular double-stranded DNA genome of approximately 8 kilo base-pairs packaged in a capsid composed of two proteins L1 and L2 . HPVs are classified into at least 170 types based on the homology of nucleotide sequences of the L1 gene , among which HPV16 and HPV18 are responsible for approximately 70% of cervical cancer cases worldwide.
The life cycle of HPV is tightly linked to the differentiation of host epithelial cells. HPV infects basal cells of stratified epithelia through small lesions, in which the viral genome is maintained as episomes without expressing capsid genes and is passed on to daughter cells. When the host cells initiate epithelial differentiation, the HPV genome starts to replicate, and infectious virions are produced and released from terminally differentiated cornified cells .
Productive replication of the HPV genome in differentiated cells requires a viral DNA helicase E1, a viral replication/transcription factor E2, and a replication origin DNA, containing specific binding sites for E1 (E1BS) and E2 (E2BS) . To initiate viral genome replication, E2 binds to the E2BS at the origin and recruits E1, leading to the formation of an E1/E2 complex at the replication origin . Then, E1 changes its conformation by binding to ATP, which causes a release of E2 from the origin. After dissociation of E2, E1 assembles into double trimers to unwind double-stranded DNA. The E1 double trimers serve as precursors for subsequent formation of double hexamers that finally function as a processive DNA helicase at replication forks .
E1 consists of four domains: an N-terminal domain (ND), a DNA-binding domain (DBD), an oligomerization domain (OD), and a helicase domain (HD) . The ND contains nuclear localization and export signals, and has a regulatory role in viral genome replication, by controlling subcellular localization of E1 . The DBD is required for E1 binding to the E1BS at the replication origin [7, 8]. The OD is responsible for E1-oligomerization [9, 10]. The HD has nonspecific DNA-binding and ATPase activities, and mediates interaction with E2 [5, 7].
Co-infection with multiple HPV types in a single cervical specimen has been reported in 30–45% of HPV-positive women [11–15]. Furthermore, several studies indicate recombination between different HPV types [16–19], which strongly suggests that a single cell can be co-infected with different HPV types in vivo.
A previous study reported that HPV45 genomes are not maintained in cultured keratinocytes co-transfected with genomes of other HPV types, such as HPV18, HPV31, and HPV39 . This study also demonstrated that while HPV31 and HPV39 genomes are stably maintained within the same cell, copy numbers of genomes of both types are extremely low compared to those in cells containing each genotype individually. These observations suggest an interference of genome replication between different HPV types. However, mechanisms underlying the replication interference have not been fully explored.
In this study, to examine simultaneous replication of HPV16 and HPV18 genomes in the same cell, we used a cell-based transient replication assay that has been used to study E1/E2-dependent HPV replication [21–26]. The HPV-negative C33A cervical cancer cell line was co-transfected with HPV16 and HPV18 genomes together with E1/E2 expression plasmids for both types, and levels of genome replication were measured by quantitative real-time PCR. We report replication interference between HPV16 and HPV18, and propose a molecular mechanism of the interference.
Expression of FLAG-tagged E1/E2s of HPV16 and HPV18 in C33A cells
We constructed expression plasmids for FLAG-tagged HPV16 E1 (F16E1), HPV16 E2 (F16E2), HPV18 E1 (F18E1), and HPV18 E2 (F18E2), and named them: pF16E1, pF16E2, pF18E1, and pF18E2, respectively. Figure 1 shows the expression of the FLAG-tagged E1/E2s in HPV-negative C33A cells transiently transfected with different mixtures of pF16E1 and pF16E2, and/or pF18E1 and pF18E2. The E1/E2 proteins of both types were detected by Western blotting with anti-FLAG antibody. The expression levels of E1/E2 of HPV18 were higher than those of HPV16. Although the expression level of HPV16 E2 was extremely low, the level was sufficient to support HPV16 replication (see below).
Replication of HPV16 or HPV18 genomes supported by homologous or heterologous E1/E2s
E1/E2s of HPV16 and HPV18 supported genome replication of both the homologous and heterologous types (Figure 2). C33A cells were transfected with circularized full-genome DNA (gDNA) of HPV16 (Figure 2A) or HPV18 (Figure 2B) together with increasing amounts of pF16E1 and pF16E2, or pF18E1 and pF18E2. Three days after transfection, low molecular weight DNA was isolated using the Hirt procedure, digested with Dpn I, and Dpn I-resistant HPV gDNA quantified by real-time PCR as previously reported [22, 25, 26]. The maximum levels of replication for HPV16 and HPV18 genomes were observed when cells were transfected with 40 ng of each pF16E1 and pF16E2 and 20 ng of each pF18E1 and pF18E2, respectively. Compared to the replication levels for HPV16 or HPV18 supported by the homologous E1/E2, replication supported by the heterologous E1/E2 was relatively inefficient.
Transfection with excess amounts of the E1/E2 expression plasmids (>80 ng of each pF16E1 and pF16E2, and >40 ng of each pF18E1 and pF18E2) decreased the replication levels for both types (Figure 2) and increased the number of detached cells (data not shown). Since E1 is known to activate a cellular DNA damage response, which results in delayed S phase [27, 28], overexpression of E1 may be toxic for C33A cells and reduce the replication efficiency. Therefore, in later experiments, we transfected cells with suboptimal amounts of the expression plasmids (<20 ng of each pF16E1 and pF16E2, and <10 ng of each pF18E1 and pF18E2).
Simultaneous replication of HPV16 and HPV18 genomes in the presence of E1/E2s of both types
Replication of HPV16 and HPV18 genomes was suppressed by co-expression of the heterologous E1/E2 (Figure 3). C33A cells were transfected with a mixture of gDNAs and E1/E2 expression plasmids for both types to mimic simultaneous replication of HPV16 and HPV18 genomes in a co-infected cell. When cells were transfected with 20 ng of each pF16E1 and pF16E2 together with 10 ng of each pF18E1 and pF18E2, the replication levels of both types were reduced to around 20%. The inhibitory effect of HPV18 E1/E2 on HPV16 replication was more pronounced than that of HPV16 E1/E2 on HPV18 replication.
Effects of heterologous E1 or E2 on HPV16/18 replication
The heterologous E1, but not E2 inhibited HPV16 and HPV18 replication (Figure 4). HPV18 E1 inhibited HPV16 replication to the level observed in the presence of E1/E2s of both types (Figure 4A). The same was true for HPV16 E1 in HPV18 replication inhibition (Figure 4B). These results clearly indicate that the replication interference between HPV16 and HPV18 is mediated by the heterologous E1, not by E2.
Effects of HPV16 E1 mutants on HPV18 replication
To examine which functional domain of HPV16 E1 is responsible for the inhibition of HPV18 replication, we constructed expression plasmids for deletion mutants of HPV16 E1 (Figure 5A), and tested their capability to inhibit HPV18 replication.
As shown in Figure 5B, the OD of HPV16 E1 was essential for the inhibition of HPV18 replication, whereas the HD is dispensable. A deletion mutant F16E1-439, which lacks the HD, inhibited HPV18 replication as efficiently as full-length F16E1. In contrast, deletion mutants F16E1-359 and F16E1-184 failed to inhibit HPV18 replication. As expected, all of the deletion mutants completely lost the ability to support HPV16 replication (data not shown). Furthermore, an amino-acid substitution mutant F16E1-Y379A, which is supposed to negate the ability of E1 to oligomerize on single-stranded DNA and to bind to the replication origin [9, 29], did not inhibit HPV18 replication. These results indicate that the OD of HPV16 E1 is responsible for the observed reduction in HPV18 replication efficiency.
Physical interaction between E1s of HPV16/18 in C33A cells
The requirement of the OD of HPV16 E1 for the inhibition of HPV18 replication strongly suggests that a physical interaction between the heterologous E1s is involved in the interference. Thus, we examined the interaction between E1s of HPV16 and HPV18 using co-immunoprecipitation assays. C33A cells were transfected with HPV18 gDNA together with expression plasmids for hexahistidine (6×His)-tagged HPV18 E1 (pH18E1), untagged HPV18 E2 (p18E2), and each of the HPV16 E1 mutants described above. Two days after transfection, F16E1 in cell lysates was immunoprecipitated with anti-FLAG antibody, followed by detection of H18E1 co-precipitated with F16E1 by Western blotting with anti-6×His antibody. H18E1 efficiently co-precipitated with F16E1 in the cell lysate (Figure 6A). Similarly H18E1 co-precipitated with F16E1 in the absence of HPV18 E2 and gDNA (Figure 6B), suggesting that the interaction is direct and not mediated by either HPV18 E2 or gDNA. H18E1 bound less efficiently to F16E1-439 and F16E1-359, but not to F16E1-184 (Figure 6A). Importantly, the OD mutant, F16E1-Y379A, showed reduced binding efficiency compared to F16E1.
The direct interaction between E1s of HPV16 and HPV18 was further confirmed by using purified E1 proteins: 6xHis-tagged HPV16 E1 (H16E1) and FLAG-tagged HPV18 E1 (F18E1). H16E1 was incubated with F18E1, and F18E1 in the mixture was immunoprecipitated with anti-FLAG antibody, followed by Western blotting with anti-6×His antibody. Clearly H16E1 co-precipitated with F18E1 (Figure 6C), indicating that HPV16 E1 directly binds to HPV18 E1.
Taken together, these results strongly suggest that HPV16 E1 interacts with HPV18 E1 through the region containing the DBD, OD, and HD, and that the OD is an important determinant for efficient interaction.
In this study using cell-based transient replication assays we found replication interference between HPV16 and HPV18 and explored the underlying molecular mechanisms. We examined replication of HPV16/18 genomes under conditions of exogenous expression of E1/E2 for both types from the Cytomegalovirus promoter because expression of E1/E2 from native HPV promoters is too weak to support HPV genome replication in C33A cells. Although these experimental conditions do not necessarily reflect a natural context of HPV transcription, the results obtained in this study provide a novel mechanistic insight into inter-type HPV replication interference, which could not be addressed in the previous study using transfection of HPV genomes alone .
The mutational analysis of HPV16 E1 indicates that the OD, which is responsible for the E1-E1 interaction [9, 10], is essential for the inhibition of HPV18 replication. In particular, the inability of the OD mutant F16E1-Y379A to inhibit HPV18 replication strongly implies that the OD-mediated interaction between HPV16 and HPV18 E1s is critical for replication interference. On the other hand, the deletion mutant F16E1-439, which lacks the HD and shows reduced binding (at a similar level to the OD mutant), still retains the capability to inhibit HPV18 replication, suggesting that the binding between HPV16 and HPV18 E1s via the HD does not contribute to the replication interference. Furthermore, because the HD is essential for helicase activity, as well as E1 binding to E2 [30–32], the results clearly indicate that the enzymatic activity of E1 and its binding to E2 are not involved in replication inhibition. It is also worth noting that the replication interference is not simply due to competition between heterologous E1/E2s for origin binding because E1/E2s of HPV16 and HPV18 supported genome replication of heterologous types (Figure 2).
A comparison of amino acid sequences between HPV16 and HPV18 E1s reveals that the OD is the most conserved region between the two (Figure 7A). The amino acid identities in the ND, DBD, OD, and HD are 46, 60, 66, and 64% homologous, respectively (Figure 7B). The high sequence similarity observed between ODs strongly supports the possibility of heterooligomer formation between the two types. Collectively, these results implicate E1 heterooligomer formation via the OD as the molecular mechanism behind replication inhibition.
We propose a model in which HPV16 and HPV18 E1 heterooligomers do not have proper configurations and are deficient in the ability to support genome replication for both HPV16 and HPV18. Since the amino acid sequence in the ND is less conserved between HPV16 and HPV18 E1s (Figure 7), it may exert a negative effect on the replication activities of E1 heterooligomers, although the exact functions of the ND in the conformation of E1 homooligomers are not yet well understood. Alternatively, it is possible that the E1 heterooligomers are unable to bind efficiently to the replication origin or unwind double-stranded DNA, and/or that they are deficient in recruiting cellular factors required for HPV replication, such as DNA polymerase alpha , replication protein A , and topoisomerase I .
Serological studies have shown that seropositivities for HPV6 and HPV11 significantly antagonize the development of HPV16-related cervical cancer [37, 38]. Interestingly, these studies also demonstrated a tendency for antagonistic interactions between HPV16 and HPV18. Seropositivity for HPV18 reduces the risk of HPV16-related cervical cancer, although statistical significance was not achieved. Although the underlying mechanism of such serological interaction is not clear, interference of genome replication between HPV16 and other HPV types may be involved, as observed in this study. It is unlikely that antibodies against HPV6, HPV11, or HPV18 capsids protect women from infection with HPV16, because antisera against these types do not cross-neutralize HPV16 in vitro . It will thus be of interest to investigate whether HPV6 and HPV11 interfere with HPV16 replication in transient replication assays such as those described here.
Interference between multiple HPV types has been also proposed in several pathological studies. Genomes of different HPV types were detected in distinct, non-overlapping areas of the same genital tissue by in situ hybridization [40–42]. When cervical tumor biopsies, in which genomes of both HPV16 and HPV18 were detected by PCR, were analyzed by fluorescence in situ hybridization, the integrated form of either HPV16 or HPV18 was detected in an individual cell . Although the genomes of HPV1 and HPV63 were detected in the same cell of a plantar wart, only a cytopathogenic effect typical of HPV63 infection was seen in the cell .
Our experimental results and previous observations reported by others indicate that interactions between different HPV types during their life cycle may affect the propagation, pathogenesis, and evolution of HPVs.
This study indicates that co-infection of a single cell with HPV16 and HPV18 results in replication interference between them, and that interaction between the heterologous E1s is responsible for the interference.
Materials and methods
Plasmids and HPV genomes
The codon-optimized E1 and E2 genes of HPV16 and HPV18 were synthesized by Life Technologies (Carlsbad, CA, USA) and cloned into the Not I site of pCMV, which had been created by removing the β-galactosidase gene from pCMVβ (Clontech, Mountain View, CA, USA). The FLAG-tag sequence was added to the 5′-terminus of each gene in pCMV by using PCR to produce pF16E1, pF16E2, pF18E1, and pF18E2. The 6xHis-tag sequence was added to the 5′-terminus of the HPV18 E1 gene in pCMV to produce pH18E1. A stop codon was introduced into pF16E1 by using PCR to produce expression plasmids for HPV16 E1 deletion mutants; pF16E1-439, pF16E1-359, and pF16E1-184 express amino acid (aa) 2 to 439, aa 2 to 359, and aa 2 to 184 of the HPV16 E1, respectively. The codon 379 of the E1 gene in pF16E1 was changed from TAC to GCA by using PCR to produce pF16E1-Y379A, which expresses HPV16 E1 with amino acid substitution of tyrosine to alanine at aa residue 379.
The circularized HPV16 and HPV18 gDNAs were prepared by in vitro self-ligation of linear viral genomes. The full-length genomes of HPV16 and HPV18 were released from the cloned vector pUC18 by digestion with Bam HI and Eco RI, respectively. The linearized genomes were incubated with T4 DNA ligase at final concentration 2.5 μg/ml of DNA for overnight at 4°C. The ligated DNAs were purified and concentrated by using the QIAprep Spin Miniprep Kit (Qiagen GmbH, Hilden, Germany).
C33A cervical carcinoma cells were cultured in Dulbecco’s modified minimal essential medium (DMEM) supplemented with 10% fetal bovine serum (FBS) and grown in 5% CO2 at 37°C.
C33A cells (1 × 106 cells) were grown in a 6-well plate for 6 h and then transfected with the expression plasmids for FLAG-tagged E1/E2 of HPV16/18 using the FuGene HD (Roche Diagnostics, Indianapolis, IN, USA). Two days after transfection the cells were lysed in SDS-sample buffer, followed by boiling of the cell lysate for 5 min. The extracted proteins were separated by SDS-PAGE and transferred to a PVDF membrane (Life Technologies). After blocking the membrane with phosphate-buffered saline (PBS) containing 0.02% Tween-20 and 5% skimmed milk, FLAG-tagged E1/E2s were probed with rabbit polyclonal anti-FLAG antibody (Sigma-Aldrich Co. St. Louis, Mo, USA) and horseradish peroxidase conjugated anti-rabbit IgG goat antibody (Santa Cruz Biotechnology, Inc., Santa Cruz, CA, USA). The immunoreactive proteins were visualized using the Pierce Western Blotting Substrate Plus (Thermo Fisher Scientific Inc. Waltham, MA, USA) and the Typhoon 9410 Image Scanner (GE Healthcare, Piscataway, NJ, USA).
Transient replication assay
C33A cells (2 × 105 cells) were grown in a 24-well plate for 6 h and then transfected with HPV gDNAs and the expression plasmids for E1/E2 together with 1 ng of pGL3-Basic (Promega, Madison, WI, USA), which lacks a replication origin for HPV, using the FuGene HD. The total amount of transfected DNA was adjusted to 400 ng with the empty vector, pCMV. The next day of the transfection, the medium was changed to DMEM containing 10% FBS. Three days after transfection low molecular weight DNA was isolated by the Hirt procedure. Briefly, 200 μl of lysis solution (10 mM Tris–HCl [pH 8.0], 10 mM EDTA [pH 8.0], and 1% SDS) was added to the cells, followed by cell lysis for 10 min at room temperature with gentle agitation. Fifty μl of 5 M NaCl was then added to the cell lysate, and incubated overnight at 4°C. The mixture was centrifuged at 50,000 × g for 30 min at 4°C to precipitate proteins and genomic DNA of the cells. The HPV gDNAs were isolated from the supernatant using the QIAamp DNA Blood Mini Kit (Qiagen GmbH), and eluted with 50 μl of elution buffer (10 mM Tris–HCl [pH 8.0] and 1 mM EDTA). To digest the transfected DNA, 2 μl of the DNA sample was incubated with 10 U of Dpn I in 20 μl of 1 × reaction buffer (New England Biolabs, Ipswich, MA, USA) for 2 h at 37°C, followed by heat inactivation of Dpn I at 80°C for 20 min. The amounts of Dpn I-resistant HPV16/18 gDNAs were quantified by real-time PCR with HPV16/18 type-specific primers and SYBR-green dye. Total 20 μl of a PCR reaction mixture containing 2 μl of the Dpn I-digested sample, 10 μl of SYBR Green Realtime PCR Master Mix (TOYOBO CO., LTD, Osaka, Japan), and 0.4 μM of each primer was subjected to real-time PCR analysis using the LightCycler 480 (Roche Diagnostics). The nucleotide sequences of primers are as follows: forward primer for HPV16, 5′-CACCTCCAGCACCTAAAGAA; reverse primer for HPV16, 5′-TTGCGTCCTAAAGGAAACTG; forward primer for HPV18, 5′-GATGTGAGAAACACACCACA; reverse primer for HPV18, 5′-GCAGTGAAGTGTTCAGTTCC; forward primer for the luciferase gene, 5′-AGGCGAACTGTGTGTGAGAG; reverse primer for the luciferase gene, TTCAGGCGGTCAACGATGAA. Each amplicon of the HPV16/18 genomes contains two Dpn I sites, whereas that of the luciferase gene has no Dpn I site. The amounts of Dpn I-resistant HPV gDNA were normalized to those of the luciferase gene.
C33A cells (1 × 106 cells) were grown in a 6-well plate for 6 h and then transfected with HPV18 gDNA, pH18E1, and p18E2, together with one of the expression plasmids for HPV16 E1 mutants, using the FuGene HD. Two days after transfection the cells were lysed in 100 μl of RIPA buffer (25 mM Tris–HCl [pH7.6], 150 mM NaCl, 1% NP-40, 1% sodium deoxycholate, and 0.1% SDS), followed by centrifugation of the cell lysate at 10,000 × g for 10 min at 4°C. The supernatant was diluted 4-fold with PBS, and precleared with 20 μl of Dynabeads protein G magnetic beads (Life Technologies) for 30 min at 4°C. The precleared lysate was further incubated with 2 μg of the rabbit polyclonal anti-FLAG antibody (Sigma-Aldrich Co.) and 20 μl of the protein G magnetic beads for 2 h at 4°C. The beads were then washed with PBS containing 0.02% Tween-20 four times, and the bound proteins were eluted by boiling the beads in 20 μl of SDS-sample buffer. The recovered proteins were resolved by SDS-PAGE and transferred to a PVDF membrane. 6×His-tagged HPV18 E1 on the membrane was probed by mouse monoclonal anti-6×His antibody (Qiagen GmbH) and detected with horseradish peroxidase conjugated anti-mouse IgG goat antibody (Santa Cruz Biotechnology, Inc.) as described above.
6×His-tagged HPV16 E1 (H16E1) protein was prepared from bacterial cells. Briefly, the H16E1 gene was cloned into pET-30 (Novagen, Madison, WI, USA), and the H16E1 protein was purified from Escherichia coli BL21(DE3) pLysS that had been transformed with the expression plasmid as described previously . FLAG-tagged HPV18 E1 (F18E1) protein was prepared from insect cells by using the baculovirus expression system (Life Technologies). Briefly, the F18E1 gene was cloned into pFastBac1 (Life Technologies), and the resultant plasmid was introduced into E. coli DH10Bac-competent cells (Life Technologies) to obtain recombinant Bacmid DNA. A recombinant baculovirus expressing F18E1 was produced in Sf9 cells transfected with the recombinant Bacmid DNA. The F18E1 protein was purified from Sf9 cells that had been infected with the recombinant baculovirus as described previously . For binding reaction, 1 μg of H16E1 and 4 μg of F18E1 were diluted with 200 μl of binding buffer (20 mM Tris–HCl [pH8.0], 150 mM NaCl, 2 mM MgCl2, and 0.01% NP-40), and incubated with 4 μl of the rabbit polyclonal anti-FLAG antibody (Sigma-Aldrich Co.) and 15 μl of the protein G magnetic beads (Life Technologies) for 1 h at 4°C. The beads were then washed with the binding buffer four times, and the bound proteins were analyzed by Western blotting as described above.
E1 binding site
E2 binding site
Dulbecco’s modified minimal essential medium
Fetal bovine serum
Howley PM, Lowy DR: Papillomaviruses and their replication. In Fields Virology Volume 2. 4th edition. Edited by: Lnipe DM, Howley PM. Philadelphia: Lippincott, Williams and Wilkins; 2001:2197-2229.
de Villiers EM: Cross-roads in the classification of papillomaviruses. Virology 2013, 445: 2-10. 10.1016/j.virol.2013.04.023
Longworth MS, Laimins LA: Pathogenesis of human papillomaviruses in differentiating epithelia. Microbiol Mol Biol Rev 2004, 68: 362-372. 10.1128/MMBR.68.2.362-372.2004
McBride AA: Replication and partitioning of papillomavirus genomes. Adv Virus Res 2008, 72: 155-205.
Schuck S, Stenlund A: Assembly of a double hexameric helicase. Mol Cell 2005, 20: 377-389. 10.1016/j.molcel.2005.09.020
Deng W, Lin BY, Jin G, Wheeler CG, Ma T, Harper JW, Broker TR, Chow LT: Cyclin/CDK regulates the nucleocytoplasmic localization of the human papillomavirus E1 DNA helicase. J Virol 2004, 78: 13954-13965. 10.1128/JVI.78.24.13954-13965.2004
Sarafi TR, McBride AA: Domains of the BPV-1 E1 replication protein required for origin-specific DNA binding and interaction with the E2 transactivator. Virology 1995, 211: 385-396. 10.1006/viro.1995.1421
Thorner LK, Lim DA, Botchan MR: DNA-binding domain of bovine papillomavirus type 1 E1 helicase: structural and functional aspects. J Virol 1993, 67: 6000-6014.
Titolo S, Pelletier A, Pulichino AM, Brault K, Wardrop E, White PW, Cordingley MG, Archambault J: Identification of domains of the human papillomavirus type 11 E1 helicase involved in oligomerization and binding to the viral origin. J Virol 2000, 74: 7349-7361. 10.1128/JVI.74.16.7349-7361.2000
Enemark EJ, Joshua-Tor L: Mechanism of DNA translocation in a replicative hexameric helicase. Nature 2006, 442: 270-275. 10.1038/nature04943
Gravitt PE, Peyton CL, Alessi TQ, Wheeler CM, Coutlée F, Hildesheim A, Schiffman MH, Scott DR, Apple RJ: Improved amplification of genital human papillomaviruses. J Clin Microbiol 2000, 38: 357-361.
Coutlée F, Gravitt P, Kornegay J, Hankins C, Richardson H, Lapointe N, Voyer H, Franco E: Use of PGMY primers in L1 consensus PCR improves detection of human papillomavirus DNA in genital samples. J Clin Microbiol 2002, 40: 902-907. 10.1128/JCM.40.3.902-907.2002
van Doorn LJ, Quint W, Kleter B, Molijn A, Colau B, Martin MT, Kravang-In , Torrez-Martinez N, Peyton CL, Wheeler CM: Genotyping of human papillomavirus in liquid cytology cervical specimens by the PGMY line blot assay and the SPF(10) line probe assay. J Clin Microbiol 2002, 40: 979-983. 10.1128/JCM.40.3.979-983.2002
Klug SJ, Hukelmann M, Hollwitz B, Düzenli N, Schopp B, Petry KU, Iftner T: Prevalence of human papillomavirus types in women screened by cytology in Germany. J Med Virol 2007, 79: 616-625. 10.1002/jmv.20863
Kondo K, Uenoyama A, Kitagawa R, Tsunoda H, Kusumoto-Matsuo R, Mori S, Ishii Y, Takeuchi T, Kanda T, Kukimoto I: Genotype distribution of human papillomaviruses in Japanese women with abnormal cervical cytology. Open Virol J 2012, 6: 277-283. 10.2174/1874357901206010277
Narechania A, Chen Z, DeSalle R, Burk RD: Phylogenetic incongruence among oncogenic genital alpha human papillomaviruses. J Virol 2005, 79: 15503-15510. 10.1128/JVI.79.24.15503-15510.2005
Varsani A, van der Walt E, Heath L, Rybicki EP, Williamson AL, Martin DP: Evidence of ancient papillomavirus recombination. J Gen Virol 2006, 87: 2527-2531. 10.1099/vir.0.81917-0
Angulo M, Carvajal-Rodríguez A: Evidence of recombination within human alpha-papillomavirus. Virol J 2007, 28: 33.
Gottschling M, Stamatakis A, Nindl I, Stockfleth E, Alonso A, Bravo IG: Multiple evolutionary mechanisms drive papillomavirus diversification. Mol Biol Evol 2007, 24: 1242-1258. 10.1093/molbev/msm039
McLaughlin-Drubin ME, Meyers C: Evidence for the coexistence of two genital HPV types within the same host cell in vitro. Virology 2004, 321: 173-180. 10.1016/j.virol.2003.12.019
Chiang CM, Ustav M, Stenlund A, Ho TF, Broker TR, Chow LT: Viral E1 and E2 proteins support replication of homologous and heterologous papillomaviral origins. Proc Natl Acad Sci USA 1992, 89: 5799-5803. 10.1073/pnas.89.13.5799
Taylor ER, Morgan IM: A novel technique with enhanced detection and quantitation of HPV-16 E1- and E2-mediated DNA replication. Virology 2003, 315: 103-109. 10.1016/S0042-6822(03)00588-9
Wang XM, Jansen KU, McClements WL: DNA replicative functions of highly-expressed, codon-optimized human papillomavirus proteins E1 and E2. J Virol Methods 2003, 108: 83-90. 10.1016/S0166-0934(02)00262-8
Lin BY, Broker TR, Chow LT: Analysis of HPV DNA replication using transient transfection and cell-free assays. Methods Mol Med 2005, 119: 331-348.
Morgan IM, Taylor ER: Detection and quantitation of HPV DNA replication by Southern blotting and real-time PCR. Methods Mol Med 2005, 119: 349-362.
Kukimoto I, Mori S, Sato H, Takeuchi T, Kanda T: Transcription factor human Skn-1a enhances replication of human papillomavirus DNA through the direct binding to two sites near the viral replication origin. FEBS J 2008, 275: 3123-3135. 10.1111/j.1742-4658.2008.06468.x
Sakakibara N, Mitra R, McBride AA: The papillomavirus E1 helicase activates a cellular DNA damage response in viral replication foci. J Virol 2011, 85: 8981-8995. 10.1128/JVI.00541-11
Fradet-Turcotte A, Bergeron-Labrecque F, Moody CA, Lehoux M, Laimins LA, Archambault J: Nuclear accumulation of the papillomavirus E1 helicase blocks S-phase progression and triggers an ATM-dependent DNA damage response. J Virol 2011, 85: 8996-9012. 10.1128/JVI.00542-11
Titolo S, Brault K, Majewski J, White PW, Archambault J: Characterization of the minimal DNA binding domain of the human papillomavirus e1 helicase: fluorescence anisotropy studies and characterization of a dimerization-defective mutant protein. J Virol 2003, 77: 5178-5191. 10.1128/JVI.77.9.5178-5191.2003
Yasugi T, Benson JD, Sakai H, Vidal M, Howley PM: Mapping and characterization of the interaction domains of human papillomavirus type 16 E1 and E2 proteins. J Virol 1997, 71: 891-899.
Masterson PJ, Stanley MA, Lewis AP, Romanos MA: A C-terminal helicase domain of the human papillomavirus E1 protein binds E2 and the DNA polymerase alpha-primase p68 subunit. J Virol 1998, 72: 7407-7419.
Sun Y, Han H, McCance DJ: Active domains of human papillomavirus type 11 E1 protein for origin replication. J Gen Virol 1998, 79: 1651-1658.
Katoh K, Standley DM: MAFFT multiple sequence alignment software version 7: improvements in performance and usability. Mol Biol Evol 2013, 30: 772-780. 10.1093/molbev/mst010
Park P, Copeland W, Yang L, Wang T, Botchan MR, Mohr IJ: The cellular DNA polymerase alpha-primase is required for papillomavirus DNA replication and associates with the viral E1 helicase. Proc Natl Acad Sci USA 1994, 91: 8700-8704. 10.1073/pnas.91.18.8700
Loo YM, Melendy T: Recruitment of replication protein A by the papillomavirus E1 protein and modulation by single-stranded DNA. J Virol 2004, 78: 1605-1615. 10.1128/JVI.78.4.1605-1615.2004
Clower RV, Fisk JC, Melendy T: Papillomavirus E1 protein binds to and stimulates human topoisomerase I. J Virol 2006, 80: 1584-1587. 10.1128/JVI.80.3.1584-1587.2006
Silins I, Wang Z, Avall-Lundqvist E, Frankendal B, Vikmanis U, Sapp M, Schiller JT, Dillner J: Serological evidence for protection by human papillomavirus (HPV) type 6 infection against HPV type 16 cervical carcinogenesis. J Gen Virol 1999, 80: 2931-2936.
Luostarinen T, af Geijersstam V, Bjørge T, Eklund C, Hakama M, Hakulinen T, Jellum E, Koskela P, Paavonen J, Pukkala E, Schiller JT, Thoresen S, Youngman LD, Dillner J, Lehtinen M: No excess risk of cervical carcinoma among women seropositive for both HPV16 and HPV6/11. Int J Cancer 1999, 80: 818-822. 10.1002/(SICI)1097-0215(19990315)80:6<818::AID-IJC4>3.0.CO;2-T
White WI, Wilson SD, Bonnez W, Rose RC, Koenig S, Suzich JA: In vitro infection and type-restricted antibody-mediated neutralization of authentic human papillomavirus type 16. J Virol 1998, 72: 959-964.
Nuovo GJ, Darfler MM, Impraim CC, Bromley SE: Occurrence of multiple types of human papillomavirus in genital tract lesions. Analysis by in situ hybridization and the polymerase chain reaction. Am J Pathol 1991, 138: 53-58.
Hinrichs S, Smith L, Ghazvini S, Kirven K, Palladino H, Spaulding D: Multiple HPV infection: microanatomy by in situ hybridization and immunohistochemistry. Mod Pathol 1992, 5: 257-261.
Christensen ND, Koltun WA, Cladel NM, Budgeon LR, Reed CA, Kreider JW, Welsh PA, Patrick SD, Yang H: Coinfection of human foreskin fragments with multiple human papillomavirus types (HPV-11, -40, and -LVX82/MM7) produces regionally separate HPV infections within the same athymic mouse xenograft. J Virol 1997, 71: 7337-7344.
Vermeulen CF, Jordanova ES, Szuhai K, Kolkman-Uljee S, Vrede MA, Peters AA, Schuuring E, Fleuren GJ: Physical status of multiple human papillomavirus genotypes in flow-sorted cervical cancer cells. Cancer Genet Cytogenet 2007, 175: 132-137. 10.1016/j.cancergencyto.2007.02.009
Egawa K, Shibasaki Y, de Villiers EM: Double infection with human papillomavirus 1 and human papillomavirus 63 in single cells of a lesion displaying only an human papillomavirus 63-induced cytopathogenic effect. Lab Invest 1993, 69: 583-588.
Kusumoto-Matsuo R, Kanda T, Kukimoto I: Rolling circle replication of human papillomavirus type 16 DNA in epithelial cell extracts. Genes Cells 2011, 16: 23-33. 10.1111/j.1365-2443.2010.01458.x
We thank Dr. Tadahito Kanda (Center of Research Network for Infectious Diseases, Riken, Tokyo, Japan) for critical reading of the manuscript. This work was supported by a grant-in-aid from the Ministry of Health, Labour and Welfare for the Third-Term Comprehensive 10-year Strategy for Cancer Control.
The authors declare that they have no competing interests.
SM and IK designed this study and drafted the manuscript. SM performed experiments. RKM and IK technically supported the experiments. SM, RKM, YI, TT, and IK revised the manuscript critically. All authors have read and approved the final manuscript.