Expression of hypoxia-inducible factor-1alpha and cell cycle proteins in invasive breast cancer are estrogen receptor related.

BACKGROUND: The transcription factor hypoxia-inducible factor-1 (HIF-1) is a key regulator of the cellular response to hypoxia. Previous studies showed that concentrations of its subunit HIF-1alpha, as a surrogate for HIF-1 activity, are increased during breast carcinogenesis and can independently predict prognosis in breast cancer. During carcinogenesis, the cell cycle is progressively deregulated, and proliferation rate is a strong prognostic factor in breast cancer. In this study we undertook a detailed evaluation of the relationships between HIF-1alpha and cell cycle-associated proteins.
METHODS: In a representative estrogen receptor (ER) group of 150 breast cancers, the expression of HIF-1alpha, vascular endothelial growth factor, the ER, HER-2/neu, Ki-67, cyclin A, cyclin D1, p21, p53, and Bcl-2 was investigated by immunohistochemistry.
RESULTS: High concentrations (5% or more) of HIF-1alpha were associated with increased proliferation as shown by positive correlations with Ki-67 (P < 0.001) and the late S-G2-phase protein cyclin A (P < 0.001), but not with the G1-phase protein cyclin D1. High HIF-1alpha concentrations were also strongly associated with p53 positivity (P < 0.001) and loss of Bcl-2 expression (P = 0.013). No association was found between p21 and HIF-1alpha (P = 0.105) in the whole group of patients. However, the subgroup of ER-positive cancers was characterized by a strong positive association between HIF-1alpha and p21 (P = 0.023), and HIF-1alpha lacked any relation with proliferation.
CONCLUSION: HIF-1alpha overexpression is associated with increased proliferation, which might explain the adverse prognostic impact of increased concentrations of HIF-1alpha in invasive breast cancer. In ER-positive tumors, HIF-1alpha is associated with p21 but not against proliferation. This shows the importance of further functional analysis to unravel the role of HIF-1 in late cell cycle progression, and the link between HIF-1, p21, and ER.

Introduction

Hypoxia is an important cellular stressor that triggers a survival program by which cells attempt to adapt to the new environment. This primarily involves adaptation of metabolism and/or stimulation of oxygen delivery. These cell-rescuing mechanisms can be conducted rapidly by a transcription factor that reacts to hypoxic conditions, the hypoxia-inducible factor-1 (HIF-1) [1]. HIF-1 stimulates processes such as angiogenesis, glycolysis and erythropoiesis [2] by activating genes that are responsible for these processes. The HIF-1 complex consists of two subunits, HIF-1α and HIF-1β. Protein concentrations of HIF-1α depend on the cellular oxygen concentration [3,4]. During normoxia the HIF-1α protein has a very short half-life owing to its continuous Von Hippel–Lindau (VHL) protein-mediated ubiquitination, which results in low protein concentrations in the cytoplasm. Hypoxia results in stabilization of the HIF-1α protein and translocation of the HIF-1 complex to the nucleus. In the nucleus HIF-1 binds to DNA of the consensus sequence 5'-RCGTG-3', the so-called hypoxia response elements in the promoters of target genes [5]. In this way HIF-1 allows the cell to adapt metabolism, increases O2 delivery and stimulates cell survival [6]. Besides hypoxia, HIF-1 can be upregulated by loss of the tumor suppressor genes PTEN (phosphatase and tensin homolog deleted on chromosome ten) [7] and loss of p53 [8], and by the overexpression of oncogenes such as HER-2/neu [9].

Cancer cells are able to survive and proliferate in extreme microenvironmental circumstances and show changes in oncogenes and tumor suppressor genes. Hypoxia and HIF-1 have been implicated in carcinogenesis and in clinical behavior of tumors. Upregulation of HIF-1α was noted during breast carcinogenesis [10], especially in the poorly differentiated pathway. Hypoxia is related to poor response to therapy in various cancer types. In invasive breast cancer, high HIF-1α concentrations were associated with poor survival in lymph node-negative patients [11]. As prognosis in breast cancer is closely related to proliferation rate [12], and poorly differentiated tumors usually exhibit high proliferation and HIF-1α overexpression, the prognostic value of HIF-1α might well be explained by a close association between HIF-1α and proliferation.

Proliferation is under the control of many proteins involved in cell cycle regulation. We proposed that HIF-1, as a master regulator for surviving hypoxia, might interact with such cell cycle-related proteins. We therefore investigated whether concentrations of HIF-1α were associated with aberrant expression of cell cycle proteins in human breast cancer. As a result, we report here that high concentrations of HIF-1α are associated with overexpression of p53 and markers of proliferation during the late S–G2 phase of the cell cycle. In the subgroup of estrogen receptor (ER)-positive cancers only a positive association between HIF-1α and p21 was noticed. Probably, in ER-positive cases, p21 causes cell cycle arrest as a response to increased HIF-1α concentrations.

Materials and methods

Patients

A representative and previously described group of 150 stage I/II breast cancer patients, diagnosed between 1985 and 1993 at the VU University Medical Center, Amsterdam, The Netherlands, was used [11]. By 'representative' we mean that tumor size, distribution of histological subtypes and lymph node status were as expected in a random group of stage I/II patients. Breast-conserving therapy or modified radical mastectomy were the applied surgical procedures for the primary tumors, and axillary dissection including at least levels I and II was performed for all patients. All surgical specimens were directly fixed in neutral 4% buffered formaldehyde.

All invasive breast carcinomas were histologically classified according to WHO criteria as one of the following: ductal (n = 129), lobular (n = 11), mucinous (n = 4), tubular (n = 3), cribriform (n = 1), medullary (n = 1), or metaplastic (n = 1). Tumors were graded in accordance with the criteria of Elston [13] as grade I (n = 35), grade II (n = 49), or grade III (n = 66). The mean age at the time of diagnosis was 60 years (range 30 to 86). The mean tumor diameter was 2.6 cm, ranging from 0.7 to 7.0 cm (according to the TNM [tumor, node, metastases] system: 45 T1, 94 T2, and 11 T3). Locally advanced breast cancers (TNM stage III) were excluded. The group included 81 (54%) lymph node-negative and 69 (46%) lymph node-positive patients. None of the patients received preoperative chemotherapy, hormonal therapy or radiotherapy.

Immunohistochemistry

Paraffin-embedded tumor tissue was derived from the archives of the Department of Pathology of the VU University Medical Center. Anonymous use of redundant tumor material for research purposes is part of the standard treatment agreement with patients in our hospital [14]. Immunohistochemistry was performed on sections 4 μm thick. After deparaffination and rehydration, sections were immersed for 30 min in methanol containing 0.3% hydrogen peroxide to block endogenous peroxidase activity. For assessment of HIF-1α the catalyzed signal amplification system (Dako, Glostrup, Denmark) was used as described previously [11]. All slides, except for HER-2/neu, were pretreated with a citrate buffer (10 mM, pH 6.0) for antigen retrieval by heating the slides in either a microwave oven or an autoclave (for details see Table 1).

Table 1

Mouse monoclonal antibodies, availability, dilution, incubation, antigen retrieval and detection method used

Antibody	Company	Dilution	Incubation	Antigen retrieval	Detection
Ki-67	Dako	1:40	o/n, 4°C	MW	ABC
Cyclin A	Novocastra	1:100	o/n, 4°C	Autoclave	ABC
Cyclin D1	Neomarkers	1:400	o/n, 4°C	Autoclave	ABC
p21	Pharmingen	1:500	o/n, 4°C	Autoclave	ABC-BT
p53	DAKO	1:50	o/n, 4°C	MW	ABC
Bcl-2	DAKO	1:50	o/n, 4°C	Autoclave	ABC-BT
ER	DAKO	1:50	o/n, 4°C	Autoclave	ABC
VEGF	R&D systems	1:40	o/n, 4°C	Autoclave	ABC
HIF-1α	Abcam	1:500	1 h, 20°C	Waterbath	CSA kit
HER-2/neu	M v/d Vijver	1:10,000	o/n, 4°C	None	ABC

Autoclave, autoclave for 20 min at 120°C; ABC, avidin-biotinyl complex; ABC-BT, biotinyl-tyramide enhancement; Mv/d Vijver, Dr M van der Vijver, Dutch Cancer Institute, Amsterdam, The Netherlands; MW, microwave in citrate buffer pH 6.0 for 10 min near to boiling; o/n, overnight; Waterbath, 45 min at 95°C.

After cooling down and preincubation with normal serum of the species of the secondary antibody, the primary antibodies were incubated as described in Table 1. For recognition of vascular endothelial growth factor (VEGF), a rabbit polyclonal antibody was used, which was detected with a pig anti-rabbit antibody (Dako). Subsequently, slides were incubated for 30 min with biotinylated secondary antibodies, followed by incubation for 1 h with 1:200 streptavidin–biotinylated horseradish peroxidase complex (Dako). For Bcl-2 and p21 staining, a biotinyl-tyramide enhancing step was introduced [15]. After a 30 min incubation of 1:1000 (instead of 1:200) streptavidin–biotinylated horseradish peroxidase complex, slides were incubated for 10 min with 1:1000 diluted biotinyl-tyramide solution with 0.01% hydrogen peroxide in phosphate-buffered saline, followed by incubation for 30 min with 1:200 streptavidin–biotinylated horseradish peroxidase complex. In all cases 3, 3-diaminobenzidine was used as chromagen and hematoxylin as counterstaining. Positive controls consisted of known immunoreactive carcinomas (VEGF, HIF-1α, ER, p53, cyclin D1, p21, HER-2/neu) or tonsil tissue (Ki-67, Bcl-2, cyclin A). Negative controls were obtained by omission of the primary antibodies from the staining procedure.

Quantification

For all cell cycle biomarkers, except Bcl-2, the percentage of positively stained nuclei of invasive tumor cells was scored blind by one experienced observer (PJvD). ER status was determined by the Histoscore, taking 100 or more as positive. HIF-1α staining was considered positive only when there was homogeneously dark nuclear staining; cytoplasmic staining was ignored. Cytoplasmic staining for Bcl-2 in invasive breast cancer epithelium was compared with adjacent normal breast tissue and scored as negative when absent, and as weak or strong when intensity was diminished or increased, respectively, compared with adjacent normal tissue. Cytoplasmic VEGF expression was assessed as moderate or strong.

Statistical methods

For statistical analysis with SPSS for Windows version 9.0.1., 1999 (SPSS Inc., Chicago, IL), the nonparametric χ2 was used to evaluate correlations between HIF-1α and cell cycle-associated proteins. For the cell cycle-related proteins we used traditional cutoff values [16] (as shown in Table 2), and for HIF-1α 5% was used as the cutoff value as described previously [11]. Parametric tests and correlation tests using the continuous data were also performed, but these yielded similar results and have therefore not been described to keep description of the statistical results as succinct as possible. Two-sided P values below 0.050 were regarded as significant.

Table 2

Association of HIF-1α expression with cell cycle-related proteins in 150 invasive human breast cancers

Protein	Cutoff value	Concentration of HIF-1α		P(χ2)
		<5%	≥5%
Ki-67	≤10%	58	13	<0.001
	>10%	41	38
Cyclin A	≤10%	67	19	<0.001
	>10%	31	32
Cyclin D1	≤10%	80	44	0.402
	>10%	19	7
p21	≤10%	89	41	0.105
	>10%	10	10
p53	≤25%	89	35	<0.001
	>25%	10	16
Bcl-2	Negative	4	5	0.025
	Moderate	35	26
	Strong	60	19

HIF, hypoxia-inducible factor.

Results

Whole group

Analyzing the whole group of patients (n = 150), there were significant and positive associations between HIF-1α and Ki-67 (P < 0.001), cyclin A (P < 0.001), and p53 (P < 0.001) (Table 2). A positive trend between high concentrations of HIF-1α and expression of p21 (P = 0.105) was noticed, and there was a significant inverse association between Bcl-2 (P = 0.025) and HIF-1α expression. No association between HIF-1α and cyclin D1 was found. In addition, both ER positivity and overexpression of p21 were positively associated with overexpression of cyclin D1 (P < 0.001) in the whole group of patients.

ER subgroups

Interestingly, subgroup analysis of ER-positive cancers (n = 52) revealed different associations (Table 3). Only p21 positivity was significantly associated with high concentrations of HIF-1α (P = 0.023). No associations for HIF-1α were found with Ki-67, cyclins A and D1, p53, and Bcl-2. In this subgroup, p21 was positively associated with cyclin D1 (P < 0.001) but not with p53. In contrast, the subgroup of ER-negative cancers (n = 98) showed strongly significant positive associations between HIF-1α on the one hand and Ki-67 (P < 0.001), cyclin A (P < 0.001), and p53 (P = 0.003) on the other. Again, loss of Bcl-2 (P = 0.048) was significantly negatively associated with high concentrations of HIF-1α, and no association between HIF-1α, p21, and cyclin D1 was found. The striking difference in biomarker expression between the ER-positive and ER-negative subgroups led us to test further whether this was associated with proliferation or with HIF-1α. In the ER-positive subgroup HER-2/neu-positivity was associated with high concentrations of HIF-1α (P = 0.035), but no association was found between HIF-1α, p53, and VEGF. Further, in this subgroup we observed low ER expression in HIF-1α-positive regions. In the ER-negative subgroup strong VEGF expression (P = 0.007), p53 accumulation (P = 0.003), and HER-2/neu-positivity (P = 0.003) were all positively associated with high concentrations of HIF-1α.

Table 3

Association of HIF-1α with cell cycle-related proteins in estrogen receptor-positive (n = 52) and estrogen receptor-negative (n = 98) breast cancers

Protein	Cutoff value	ER-positive			ER-negative
		HIF-1 α		P(χ2)	HIF-1 α		P(χ2)
		<5%	≥5%		<5%	≥5%
Ki-67	≤10%	24	7	0.624	34	6	<0.001
	>10%	15	7		26	32
Cyclin A	≤10%	28	9	0.756	39	10	<0.001
	>10%	10	4		21	28
Cyclin D1	≤10%	25	9	0.736	55	35	0.938
	>10%	14	4		5	3
p21	≤10%	33	7	0.023	56	34	0.497
	>10%	6	6		4	4
p53	≤25%	36	11	0.415	53	24	0.003
	>25%	3	2		7	14
Bcl-2	Negative	0	0	0.609	4	5	0.048
	Moderate	12	5		23	21
	Strong	27	8		33	11
VEGF	Weak	8	2	0.685	21	4	0.007
	Strong	31	11		39	34
HER-2/neu	Negative	36	9	0.035	55	26	0.003
	Positive	3	4		5	12

ER, estrogen receptor; HIF, hypoxia-inducible factor; VEGF, vascular endothelial growth factor.

p53 subgroups

To exclude the possibility that the data for the ER subgroups were dependent on p53 status, we also performed subgroup analysis based on p53 status (Table 4). In short, the subgroup assumed to be 'wild-type' p53 was characterized by different associations from the subgroup of ER-positive cases.

Table 4

Association of HIF-1α with cell cycle-related proteins in WT-p53 (n = 124) and M-p53 (n = 26) breast cancers

Protein	Cutoff value	'Wild type' p53			'Mutated' p53
		HIF-1 α		P(χ2)	HIF-1 α		P(χ2)
		<5%	≥5%		<5%	≥5%
Ki-67	≤10%	55	12	0.006	3	1	0.264
	>10%	34	23		7	15
Cyclin A	≤10%	62	15	0.004	5	4	0.192
	>10%	26	20		5	12
Cyclin D1	≤10%	71	31	0.248	9	13	1.00
	>10%	18	4		1	3
p21	≤10%	80	28	0.139	9	13	1.00
	>10%	9	7		1	3
Bcl-2	Negative	3	3	0.273	1	2	0.132
	Moderate	31	15		4	11
	Strong	55	17		5	2
VEGF	Weak	28	5	0.051	1	1	1.00
	Strong	61	30		9	15
HER-2/neu	Negative	82	27	0.021	9	8	0.037
	Positive	7	8		1	8

aFisher Exact Test when appropriate. HIF, hypoxia-inducible factor; VEGF, vascular endothelial growth factor; WT-p53, probably wild type p53; M-p53, probably mutated p53.

Lymph node status subgroups

Because in our former study we found an independent prognostic value for HIF-1α only in lymph node-negative breast cancers, we analyzed the subgroups of lymph node-negative (n = 81) and lymph node-positive cases (n = 69) separately (Table 5). Positive significant associations were found in the subgroup of lymph node-negative cancers between HIF-1α and Ki-67 (P < 0.001), cyclin A (P < 0.001), p21 (P = 0.049), and p53 (P = 0.001). Also in this subgroup Bcl-2 (P = 0.008) was significantly inversely associated with HIF-1α. No association was found for cyclin D1. In the subgroup of lymph node-positive cancers, Ki-67 (P = 0.035) and p53 (P = 0.042) revealed a positive association with HIF-1α. No relation with HIF-1α was found for cyclins A and D1, p21, and Bcl-2.

Table 5

Association of HIF-1α with cell cycle-related proteins in lymph node-negative (n = 81) and lymph node-positive (n = 69) breast cancers

Protein	Cutoff value	Lymph node-negative			Lymph node-positive
		HIF-1 α		P(χ2)	HIF-1 α		P(χ2)
		<5%	≥5%		<5%	≥5%
Ki-67	≤10%	36	9	<0.001	22	4	0.035
	>10%	15	21		26	17
Cyclin A	≤10%	40	10	<0.001	27	9	0.305
	>10%	10	20		21	12
Cyclin D1	≤10%	40	25	0.593	40	19	0.438
	>10%	11	5		8	2
p21	≤10%	47	23	0.049	42	18	0.839
	>10%	4	7		6	3
p53	≤25%	47	21	0.009	42	14	0.042
	>25%	4	9		6	7
Bcl-2	Negative	0	3	0.008	4	2	0.459
	Moderate	17	15		18	11
	Strong	34	11		26	8

HIF, hypoxia-inducible factor.

Ductal type subgroup

To exclude confounding mechanisms based on the mixed group of different types of breast cancer, we also performed the statistical analysis described above on the subgroup of ductal type of invasive breast cancers (n = 129), as shown in Tables 6 and 7. In short, the same associations were found as described for the group of 150 patients.

Table 6

Association of HIF-1α expression with cell cycle-related proteins in all ductal type (129 of 150) invasive human breast cancers

Protein	Cutoff value	Concentration of HIF-1α		P(χ2)
		<5%	≥5%
Ki-67	≤10%	44	11	0.001
	>10%	39	35
Cyclin A	≤10%	52	16	0.002
	>10%	30	30
Cyclin D1	≤10%	67	39	0.564
	>10%	16	7
p21	≤10%	75	36	0.057
	>10%	8	10
p53	≤25%	68	25	0.001
	>25%	15	21
Bcl-2	Negative	4	5	0.042
	Moderate	29	23
	Strong	50	17

HIF, hypoxia-inducible factor.

Table 7

Association of HIF-1α with cell cycle-related proteins in only ductal carcinoma, subdivided into estrogen receptor-positive (n = 46) and estrogen receptor-negative (n = 83) breast cancers

Protein	Cutoff value	Estrogen receptor-positive			Estrogen receptor-negative
		HIF-1 α		P(χ2)	HIF-1 α		P(χ2)
		<5%	≥5%		<5%	≥5%
Ki-67	≤10%	20	5	0.730	24	6	0.002
	>10%	15	6		24	29
Cyclin A	≤10%	24	7	0.717	28	9	0.003
	>10%	10	4		20	26
Cyclin D1	≤10%	22	7	0.100	45	32	0.693
	>10%	13	4		3	3
p21	≤10%	29	5	0.022	46	31	0.235
	>10%	6	6		2	4
p53	≤25%	29	7	0.175	39	18	0.008
	>25%	6	4		9	17
Bcl-2	Negative	0	0	0.477	4	5	0.141
	Moderate	11	5		18	18
	Strong	24	6		26	11
VEGF	Weak	8	2	1.00	18	3	0.003
	Strong	27	9		30	32
HER-2/neu	Negative	33	8	0.080	43	23	0.008
	Positive	2	3		5	12

aFisher Exact Test when appropriate. HIF, hypoxia-inducible factor; VEGF, vascular endothelial growth factor.

Discussion

In this study we found positive associations between HIF-1α and the cell cycle-related proteins cyclin A, Ki-67, and p53 in invasive human breast cancers. These associations were most evident in the lymph node-negative cases and might therefore contribute to the poor prognosis of HIF-1α-positive cancers described previously [11]. Further, the ER subgroups showed differential expression of biomarkers, suggesting an interaction between HIF-1 and ER.

In general, the expression of cyclin A and Ki-67 indicates that cells are in the S or G2 phase. Cyclin A expression is stimulated by the protein-tyrosine phosphatase cdc25A [17] and is associated with undifferentiated and ER-negative breast tumors heralding poor prognosis [18,19]. It is common to use protein concentrations of Ki-67 as a proliferation marker although its function is unknown; it is present at highest concentration in the S phase but also in the G1–G2 phase [20]. Like cyclin A, Ki-67 overexpression denotes a high proliferation rate and thus poor prognosis. Our data show that high concentrations of HIF-1α are associated with high concentrations of cyclin A and Ki-67 as markers of proliferation.

The association of HIF-1 with proliferation has been noted before [10], but it is still not fully understood [21,22]. The main question is whether HIF-1 is acting on, or is a reaction to, tumor proliferation. The latter mechanism assumes that unorganized rapidly growing tumors will outgrow their own vasculature, leading to a lack of oxygen supply, necessitating adaptation by switching to anaerobic metabolism and induction of angiogenesis. Because HIF-1 has a crucial role in these latter processes, it could be postulated that rapidly proliferating tumors need HIF-1. In this light the association between HIF-1 and proliferation is more or less epigenetic or due to tumor necrosis. According to the former mechanism, primary HIF-1 overexpression might also lead to tumor proliferation. One argument for this hypothesis is based on the observation that HIF-1α expression is not restricted to necrotic tumor areas. Another argument might be the influence of oncogenes (such as HER-2/neu or Bcl-6), tumor suppressor genes (such as von Hippel–Lindau [tumor suppressor gene] protein [pVHL] or PTEN), or growth factors (such as IGF-2) on the protein concentrations of HIF-1α [7,9,23-26]. These tumorigenic mechanisms also stimulate proliferation. In addition, the recent demonstration that pulmonary artery fibroblasts, when exposed to hypoxia, stimulate the proliferation of adjacent pulmonary artery smooth muscle cells by means of hypoxia-regulated genes indicates a stimulating role for HIF-1 in the cell cycle machinery [27].

In contrast, recent work from Goda and colleagues [28] showed in two different primary differentiated cell types that HIF-1 is necessary for the induction of growth arrest during hypoxia. HIF-1 alters the cell cycle during hypoxia by increasing the concentrations of cyclin-dependent kinase inhibitors p21 and p27. In addition, hypophosphorylation of retinoblastoma proteins is HIF-1 dependent. Goda and colleagues [28] also showed that cells lacking the HIF-1α gene had an increased progression into S phase. These in vitro data are logical in physiologic circumstances but do not comply with our observations in human cancers. Thus, it is difficult to say whether these mechanisms also occur in human breast cancer. More possibly, it might be postulated that cancer cells have lost control over the cell cycle and its potential interplay with HIF-1α.

Subgroup analyses based on ER status revealed that only in ER-positive cases positivity for p21 was associated with high concentrations of HIF-1α, without correlation between HIF-1 and proliferation. This points to an intact feedback loop in ER-expressing cells in which p21 might cause cell cycle arrest as a response to increased HIF-1α concentration, which might be regulated by cyclin D1 [29]. In contrast, in ER-negative cases, a positive association between HIF-1 on the one hand and Ki-67, cyclin A, p53, and loss of Bcl-2 on the other was noted. Apparently, the p21 feedback loop is not functional in ER-negative cells. In addition, in the ER-positive cases no association for HIF-α with VEGF and p53 could be demonstrated, which was opposite to the observation in the ER-negative subgroup. These findings suggest that the different associations in both ER subgroups cannot be attributed only to a different proliferation rate. We excluded the option that the p53 status might be the underlying cause for these differences, as shown in Table 4. It is therefore tempting to suggest that these differences might be caused by an interaction between HIF-1 and ER. Little is known about the interaction between HIF-1 and ER, but an almost significant positive association was found in endometrial cancer [30] but not in breast cancer [11,31]. In prostate cancer the presence of the androgen receptor seems necessary to potentiate the angiogenic effects of HIF-1α, although this effect is mediated by the epidermal growth factor/phosphatidylinositol 3'-kinase/protein kinase B pathway [32]. In two studies it was shown that hypoxia downregulates ER in breast cancer cell lines [33,34]. More studies are therefore merited to investigate the interaction between ER and HIF-1.

Most knowledge about the interaction between HIF-1 and the cell cycle has been gathered around p53. Some of this interplay between p53 and HIF-1 was defined by An and colleagues [35], who showed that during hypoxia p53 could not stabilize without the presence of HIF-1α. Even a direct association between p53 and HIF-1α was shown by co-immunoprecipitation in hypoxic cells. Subsequently, it was shown that p53 depends on HIF-1α when it initiates apoptosis during hypoxia [21]. In contrast, Ravi and colleagues [8] showed that the concentration of HIF-1α increased when no p53 was present in tumor cells that responded to hypoxia. HIF-1 and p53 can therefore be seen as competitors because both are upregulated by hypoxia. Whereas HIF-1 maintains homeostasis, p53 is known to induce apoptosis. However, HIF-1 might also induce apoptosis in concert with p53 [36] and through NIP3 [37]. Other factors influencing the balance between p53 and HIF-1 are competition for the cofactor p300 [38] and MDM-2 (murine double minute-2) degradation of HIF-1α through p53 [8]. Thus, a loss of wild-type p53 might be associated with increased tumor growth during hypoxia because of diminished apoptosis and augmented HIF-1-induced transcriptional activation of VEGF. Indeed, the positive association between VEGF and the accumulation of p53, which is associated with p53 mutation, has been noted in breast cancer [39].

In the present study we found a positive association between the accumulation of p53 with HIF-1α and that of p53 with VEGF (the positive association of HIF-1α and VEGF has been described elsewhere [11]). The p53/HIF-1 data are in concordance with those of Zhong and colleagues [22], who noted this association in a mixed group of colon and breast cancer patients. In contrast, in lymph node-positive breast cancer and epithelial ovarian cancer no relation between p53 and HIF-1α was found [31,40]. Interestingly, we noticed that a classical association of HIF with proliferation and VEGF is true in wild-type p53 but not in the 'mutated' subgroup (assuming that more than 25% nuclear p53 accumulation points to a p53 mutation). Thus, these data imply that HIF needs wild-type p53 to exert its downstream effects.

Combined high expression of p21 and cyclin D1 was positively associated with high differentiation and low proliferation in various carcinomas including breast cancer [29,41]. Interestingly, in this study, increased concentrations of cyclin D1 corresponded to high concentrations of p21 (as previously [29]), but not of HIF-1α. Many investigators have searched for an explanation of why cyclin D1 becomes upregulated in breast cancer. The most plausible explanation is the assumption that an amplification or translocation of the cyclin D1 gene is responsible, but other mechanisms also seem to be involved because of the low incidence of cyclin D1 amplification. It has been shown that cyclin D1 exerts the effects of ER [42], confirming the importance of cyclin D1 in breast cancer. The results reported here might provide circumstantial evidence that upregulation of cyclin D1 might be caused indirectly either by hypoxia or oncogenes that can stimulate HIF-1 and thereby p21. In fact, some specific pVHL-deficient renal cell carcinoma cell lines showed such an association, although no feasible mechanism was described [43].

BCL-2 is known as an inhibitor of apoptosis. In this study we found an inverse association between HIF-1α and BCL-2. This is in contradiction of an earlier study on melanoma cell lines that showed that BCL-2 augments the angiogenic potential of HIF-1 by means of increased VEGF transcription and prolonged VEGF mRNA stabilization [44]. However, another paper suggested that VEGF itself stimulated BCL-2 expression in breast cancer [45]. Meanwhile, loss of BCL-2 fits the model in which upregulation of HIF-α is associated with breast cancer aggressiveness, because a loss of BCL-2 is associated with tumor aggressiveness [46]. We described previously that the rate of apoptosis and the concentrations of HIF-1α are both increased in aggressive breast cancers [47]. This could be an epigenetic phenomenon, but other studies do indeed point to a direct apoptotic effect of HIF-1 when the cell loses control of homeostasis despite HIF-1 activation [48].

Conclusion

HIF-1α overexpression is associated with increased proliferation, which might explain the adverse prognostic impact of increased concentrations of HIF-1α in invasive breast cancer. In ER-positive tumors HIF-1α is associated with p21, but not with proliferation. This shows the importance of further functional analysis to unravel the role of HIF-1 in late cell cycle progression, and the link between HIF-1, p21, and ER.

Competing interests

None declared.

Authors' contributions

RB was responsible for generating the hypothesis, collecting patient material, immunostaining, statistics, and writing the manuscript. PJvD was responsible for generating the hypothesis, classification of immunostaining, and correcting the manuscript. PvdG was responsible for immunostaining and correcting the manuscript. AS and AEG were responsible for generating the hypothesis and correcting the manuscript. EvdW was the study director, and was responsible for generating the hypothesis and correcting the manuscript.

Abbreviations

ER = estrogen receptor; HIF-1 = hypoxia-inducible factor-1; PTEN = phosphatase and tensin homolog deleted on chromosome ten; pVHL = von Hippel–Lindau (tumor suppressor gene) protein; VEGF = vascular endothelial growth factor.