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Annals of Oncology 13: 15981604, 2002
Original article DOI: 10.1093/annonc/mdf248
2002 European Society for Medical Oncology
Clinical implications of expression of ETS-1 related to
angiogenesis in uterine cervical cancers
J. Fujimoto*, I. Aoki, H. Toyoki, S. Khatun & T. Tamaya
*Correspondence to: Dr J. Fujimoto, Department of Obstetrics andGynecology, Gifu University School of Medicine, 40 Tsukasa-machi,Gifu City 500-8705, Japan. Tel: +81-58-267-2631;
Fax: +81-58-265-9006; E-mail: [email protected]
Department of Obste trics and Gynecology, Gifu Univers ity School of Medicine, Gifu City, Japan
Received 6 November 2001; revised 18 February 2002; accepted 26 March 2002
Background: Angiogenesis is essential for development, growth and advancement of solid tumors.
ETS-1 has been recognized as a candidate for tumor angiogenic transcription factor. This prompted us
to study the clinical implications of ETS-1-related angiogenesis in uterine cervical cancers.
Patients and methods: Fifty patients underwent curative resection for uterine cervical cancers. The
patients prognoses were analyzed with a 24-month survival rate. In the tissue of 60 uterine cervical
cancers, the levels of ets-1 mRNA, vascular endothelial growth factor (VEGF), basic fibroblast growth
factor (bFGF), platelet-derived endothelial cell growth factor (PD-ECGF) and interleukin (IL)-8 were
determined by competitive reverse transcriptionpolymerase chain reaction using recombinant RNA
and enzyme immunoassay, and the localization and counts of microvessels were determined by
immunohistochemistry.
Results: There was a significant correlation between microvessel counts and ets-1 gene expression
levels in uterine cervical cancers. Immunohistochemical staining revealed that the localization of
ETS-1 was similar to that of vascular endothelial cells. The level of ets-1 mRNA correlated with the
levels of PD-ECGF and IL-8 among angiogenic factors. Furthermore, the prognosis of the 25 patients
with high ets-1 mRNA expression in uterine cervical cancers was extremely poor, while the 24-month
survival rate of the other 25 patients with low ets-1 mRNA expression was 92%.
Conclusions: ETS-1 might be a prognostic indicator as an angiogenic mediator in uterine cervical
cancers.
Key words: angiogenesis, ets-1, IL-8, PD-ECGF, uterine cervical cancer
Introduction
Angiogenesis is essential for development, growth and
advancement of solid tumors [1]. The angiogenic factors
vascular endothelial growth factor (VEGF), basic fibroblast
growth factor (bFGF), platelet-derived endothelial cell growth
factor (PD-ECGF), identified with thymidine phosphorylase
(TP), and interleukin (IL)-8 work on angiogenesis in uterine
cervical cancers [28]. VEGF, particularly its VEGF165 and
VEGF121 isomers, was dominantly expressed in cancer cells,
especially in adenocarcinomas, but its levels did not correlate
with patient prognosis [2]. Basic FGF was expressed in both
cancer and interstitial cells of uterine cervix, and its levels cor-
related with clinical stage, but not in an obvious manner with
patient prognosis [3]. PD-ECGF was dominantly expressed in
interstitial cells of uterine cervical cancers, and its levels cor-
related with patient prognosis in the primary tumor of uterine
cervical cancers, especially in the metastatic lymph nodes
[4, 5]. Most noteworthy, serum PD-ECGF can be used as a
tumor marker of both squamous cell carcinoma and adeno-
carcinoma of the uterine cervix [6]. IL-8 was supplied from
tumor-associated macrophages infiltrated near cancer cells,
and its levels correlated with patient prognosis [7]. Therefore,
if PD-ECGF and IL-8 can be suppressed as a tumor dormancy
therapy, patient prognosis should be remarkably improved
without the severe side effects of chemotherapy. Because
chemotherapy is often not so specific to cancer cells, it
produces severe side effects even on normal cells, especially
bone marrow cells. On the other hand, tumor dormancy
therapy is specific to the rapidly growing vascular endothelial
cells in tumors, without an effect on slow-growing vascular
endothelial cells and other normal cells. However, if an angio-
genic factor is suppressed by tumor dormancy therapy for a
long period, another angiogenic factor might be induced by an
alternatively linked angiogenic pathway; this is recognized as
tolerance.
During angiogenesis, ETS-1 is strongly expressed in vascu-
lar endothelial cells and the adjacent interstitial cells [8]. Once
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angiogenesis has finished, ETS-1 expression is distinctly
down-regulated [9, 10]. The representative angiogenic factors
VEGF and bFGF immediately induce ETS-1 expression in the
early stage of angiogenesis, while the inhibition of ETS-1
expression leads to suppression of angiogenesis [11, 12]. The
proteases urokinase type-plasminogen activator (u-PA), and
matrix metalloprotease (MMP)-1, -3 and -9 conserve an
ETS-binding motif, and transcription factor ETS-1 converts
vascular endothelial cells to angiogenic phenotypes by induc-
ing u-PA, MMP-1, MMP-3 and MMP-9 and integrin 3 gene
expression [13, 14]. This status prompted us to study whether
transcription factor ETS-1 works as an angiogenic mediator,
and, if so, which angiogenic factors link to ETS-1 for angio-
genesis in uterine cervical cancers. The aim of the study was to
formulate an efficient tumor dormancy therapy.
Patients and methods
Patients
Consent for the following studies was obtained from all patients and theResearch Committee for Human Subjects, Gifu University School of
Medicine. Of 60 patients (stage Ib, 15 cases; stage II, 20 cases; stage III,
20 cases; and stage IVa, 5 cases) ranging from 31 to 87 years of age, 50
underwent curative resection at the Department of Obstetrics and
Gynecology, Gifu University School of Medicine, between October 1995
and December 1998; this resulted in macroscopic disease-free status. The
prognosis for these 50 patients was analyzed with a 24-month survival
rate. None of the patients had received any therapy before the cervical
cancer tissue was taken. A section of each uterine cervical cancer tissue
was snap-frozen in liquid nitrogen to determine levels of ets-1 mRNA,
VEGF, bFGF, PD-ECGF and IL-8, and a neighboring piece of tissue was
submitted for histopathological analysis, including immunohistochemical
staining for ets-1 and factor VIII-related antigen. The clinical stage of the
uterine cervical cancers was determined according to the International
Federation of Obstetrics and Gynecology (FIGO) classification [15].
Preparation of internal standard recombinant RNA
Internal standard recombinant RNA (rcRNA) was prepared for competit-
ive reverse transcriptionpolymerase chain reaction (RTPCR) and South-
ern blot analysis [16] as follows. Deoxynucleic acid construction of the
internal standard was originated and synthesized by PCR from aBamHI/
EcoRI-ligated fragment of V-erbB (Clontech Laboratories, Palo Alto, CA,
USA) with two sets of oligonucleotide primer sequences. The sequences for
the first set of primers for ets-1 mRNA (MIMIC ets-1-5 and MIMIC ets-1-
3) in the first PCR reaction were as follows: MIMIC ets-1-5, 5-ATGG-
AGTCAACCCAGCCTATCGCAAGTGAAATCTCCTCCG-3; MIMIC
ets-1-3, 5-CCATGCACATGTTGTCTGGGTCTGTCAATGCAGTTT-GTAG-3 [17, 18]. The sequences for the second set of primers for ets-1
mRNA (MIMIC ets-1-P and ets-1-3) in the secondary PCR reaction were
as follows: MIMIC ets-1-P, 5-TAATACGACTCACTATAGGATGG-
AGTCAACCCAGCCTAT-3 ; ets-1-3, 5-CCATGCACATGTTGTCT-
GGG-3. The first PCR cycle was conducted in a final volume of 50 l
containing PCR buffer (50 mM KCl, 10 mM TrisHCl pH 8.3, 1.5 mM
MgCl2), 0.2 mM deoxyribonucleoside triphosphates (dNTPs), 2 ng of
BamHI/EcoRI-ligated DNA fragment of V-erbB, 10 pmol each of the first
set of PCR primers and 2.5 U Amplitaq DNA polymerase (Perkin-Elmer
Cetus, Norwalk, CT, USA). The second PCR cycle was conducted in a
final volume of 100 l containing PCR buffer, 0.2 mM dNTPs, 50 pg of
the first PCR products, 20 pmol each of the second set of PCR primers and
5 U Amplitaq DNA polymerase. The mixture was amplified for 28 cycles
of PCR for 45 s at 94C for denaturing, 45 s at 55C for annealing and 90 s
at 72C for extension in a DNA Thermal Cycler (Perkin-Elmer Cetus).
The second PCR products were purified with a Gene Clean kit (Bio 101
Inc, La Jolla, CA, USA) and transcribed with 100 U T7 RNA polymerase
(Gibco-BRL, Gaithersberg, MD, USA) in a final volume of 100 lcontaining T3/T7 buffer (40 mM TrisHCl, pH 8.0, 8 mM MgCl2, 2 mM
spermidine-(HCl)3, 25 mM NaCl), 0.1 M dithiothreitol (DTT), 10 mM
ribonucleotide triphosphate, 40 U RNase inhibitor (Promega, Madison,
WI, USA), 20 mM template DNA and 10 Ci of DNase (Takara Shuzo,
Kyoto, Japan) at 37C for 5 min to remove the DNA template. The pro-
ducts were subsequently extracted with water-saturated [-32P]UTP (New
England Nuclear, Boston, MA, USA) as a tracer. The reaction was incu-
bated at 37C for 1 h, and then treated with 70 U of RNase-free phenol/
chloroform and passed through a Sephadex G50 II column (Boehringer
Mannheim, Mannheim, Germany). The amount of transcribed internal
marker was calculated from the total radioact ivity of the transcribed RNA.
Competitive RTPCR Southern blot analysis
Total RNA was isolated from tissues using the acid guanidium thio-
cyanatephenolchloroform extraction method [19].
To obtain a standard curve each time, the total RNA (3 g) and a series
of diluted recombinant RNA for ets-1 mRNA (1100 fmol) were reverse
transcribed for 1 h at 37C in a 20 l volume with a mixture of 200 U
Moloney murine leukemia virus reverse transcriptase (MMLV-RTase;
Gibco-BRL) and the following reagents: 50 mM TrisHCl, pH 8.3,
75 mM KCl, 3 mM MgCl2, 40 U RNAsin (Toyobo, Osaka, Japan), 10 mM
DTT, 0.5 mM dNTPs and 30 pmol 3-end specific primer as detailed
below. The reaction was incubated for 5 min at 94C to inactivate the
MMLV-RTase.
The sequences of primers to amplify the genes of ets-1 (ets-1-5 and
ets-1-3) were: ets-1-5, 5-ATGGAGTCAACCCAGCCTAT-3 (exon 5);
ets-1-3, 5-CCATGCACATGTTGTCTGGG-3 (exon 6). The sizes ofPCR products for ets-1 mRNA and its internal standard rcRNA were
288 bp and 440 bp, respectively. PCR with reverse-transcribed RNAs as
templates (1 l) and 5 pmol of each specific primer was carried out using
a DNA Thermal Cycler with 0.5 U Amplitaq DNA polymerase in a buffer
containing 50 mM KCl, 10 mM TrisHCl, pH 8.3, 1.5 mM MgCl2 and
0.2 mM dNTPs in a 20 l volume. Thirty cycles of amplification for ets-1
mRNA were performed at 94C for 45 s for denaturing, 55C for 45 s for
annealing and 72C for 90 s for extension.
Amplified PCR products (8 l) were electrophoresed with 1.2% agarose
gel in a 100 V constant voltage field. PCR products were capillary-
transferred to an Immobilon transfer membrane (Millipore Corp., Bed-
ford, MA, USA) for 16 h. The membrane was dried at 80C for 30 min,
then ultra violet (UV)-irradiated to fix PCR products tightly. These PCR
products were prehybridized in buffer (1 M NaCl, 50 mM TrisHCl, pH7.6, 1% sodium dodecyl sulfate) at 42C for 1 h, and hybridized in the
same solution with the biotinylated oligodeoxynucleotide probe (ets-1-DT,
5-TGGTATTGAGCATGCCCAGT-3 for the ets-1 gene), synthesized
from the sequences of ets-1 cDNA between the specific primers, and the
corresponding biotinylated internal standard gene-specific oligonucleo-
tide probe (MIMIC-DT, 5-GCAGATGAGTATCTTGTCCC-3 ) simul-
taneously to check gene specificity at 65C overnight. They were also
hybridized with the biotinylated ets-1-5 probe (10 pmol/ml) to determine
the signal intensity under the same conditions. Specific bands hybridized
with the biotinylated probes were detected with Plex Luminescent Kits
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(Millipore Corp.), and X-ray film was exposed on the membrane at room
temperature for 10 min. The quantification of Southern blot was carried
out with Bio Image (Millipore, Ann Arbor, MI, USA).
In the competitive RTPCR Southern blot analysis for ets-1 mRNA,
only two predicted sizes of DNA fragment were detected with ets-1-DT
and ets-1-5 simultaneously to check specificity and determine quantity,
respectively. As a negative control, no ets-1 mRNA was detected without
reverse transcription in 30 cycles of PCR. The levels of ets-1 mRNA were
determined using a standard curve and a serial dilution of rcRNA in
competitive RTPCR Southern blot analyses, as shown in Figure 1.
Immunohistochemistry
Four-micrometre sections of formalin-fixed, paraffin-embedded tissues
of uterine endometrial cancers were cut with a microtome and dried over-
night at 37C on a silanized-slide (Dako, Carpinteria, CA, USA). Samples
were deparaffinized in xylene at room temperature for 80 min and washedwith a graded ethanol/water mixture and then with distilled water. The
samples for ETS-1 were soaked in a citrate buffer, and then microwaved at
100C for 10 min, and those for factor VIII-related antigen were treated
with 0.3 g/ml trypsin in phosphate buffer at room temperature for
20 min. The protocol for a DAKO LSAB2 Kit, Peroxidase (Dako), for
immunohistochemical staining was followed for each sample. In this
protocol, rabbit anti-human ETS-1 (C-20; Santa Cruz Biotechnology,
Santa Cruz, CA, USA) and rabbit anti-factor VIII-rela ted antigen (Zymed,
San Francisco, CA, USA) were used as the first antibodies at dilutions of
1:2000 and 1:2, respectively. The addition of the first antibody, rabbit
anti-human ETS-1 or rabbit anti-factor VIII-related antigen, was omitted
in the protocols for negative controls of ETS-1 or factor VIII-related
antigen, respectively.
Vessels were counted in the five highest density areas at magnification
200 (0.785 mm2 per field). Microvessel counts were expressed as the
mean numbers of vessels in these areas [20]. Microvessel density was
evaluated by counting microvessels.
Enzyme immunoassay for determination of bFGF, VEGF,PD-ECGF and IL-8 antigens
All steps were carried out at 4C. Tissues of uterine cervical cancers
(wet weight 1020 mg) were homogenized in HG buffer (5 mM TrisHCl,
pH 7.4, 5 mM NaCl, 1 mM CaCl2, 2 mM ethyleneglycol-bis-[-amino-
ethyl ether]-N,N,N,N- tetraacetic acid, 1 mM MgCl2, 2 mM DTT,
25 g/ml aprotinin, and 25 g/ml leupeptin) with a Polytron homogenizer
(Kinematics, Luzern, Switzerland). This suspension was centrifuged in a
microfuge at 10000 g for 3 min to obtain the supernatant. The protein
concentration of samples was measured by the method of Bradford [21] to
standardize VEGF, bFGF, PD-ECGF and IL-8 antigen levels.
Basic FGF, VEGF and IL-8 antigen levels in the samples were
determined by a sandwich enzyme immunoassay using a Human bFGF
Quantikine kit, a Human VEGF Quantikine kit and a Human IL-8
Quantikine kit (all from R&D Systems, Minneapolis, MN, USA), respect-
ively. PD-ECGF antigen levels were determined by the method described
by Nishida et al. [22]. The levels of bFGF, VEGF, PD-ECGF and IL-8
were standardized with the corresponding cellular protein concentrations.
Statistics
Survival curves were calculated using the KaplanMeier method and
analyzed by the log-rank test. The levels of ets-1 mRNA, VEGF, bFGF,
PD-ECGF and IL-8 were measured from three samples taken from each
tissue, and the assay for each sample was carried out in triplicate. Differ-
ences were considered significant at P
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Figure 2. Immunohistochemical staining for ETS-1 and factor VIII-
related antigen in uterine cervical cancers. A case of uterine cervical
cancer. Rabbit anti-human ETS-1 (Santa Cruz Biotechnology) and mouse
anti-human factor VIII-related antigen (Zymed) were each used at
dilutions of 1:2000 and 1:2, respectively, as the first antibodies. Original
magnification: 200.
Figure 3. Correlation between microvessel counts and ets-1 mRNA
levels in uterine cervical cancers.
Figure 4. Levels of ets-1 mRNA in uterine cervical cancers, classified
according to clinical stage (FIGO). Each level is the mean of nine
determinations. Alive and deceased cases are shown as open and closed
circles, respectively.
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There was a significant correlation between ets-1 mRNA
levels and PD-ECGF (P
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the major angiogenic factors along with suppression of ETS-1
recruitment might be more effective as a tumor dormancy
therapy than as mere suppression of major angiogenic factors.
A specific inhibitor for ETS-1, transdominant mutant ETS-1,
has already been shown to act as a dominant negative
molecule, and can be used as an efficient tool for angiogenic
inhibition [38].
Acknowledgements
This study was supported in part by funds from the following
Ministry of Health and Welfare programs of the Japanese
Government: Grant for Scientific Research Expenses for
Health and Welfare Programs, Foundation for Promotion of
Cancer Research, and Grant-in-Aid for the Second Term
Comprehensive 10-year Strategy for Cancer Control. The
authors wish to thank Mr John Cole for proofreading this
manuscript.
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