Regulatory Peptides 120 (2004) 69 – 75
www.elsevier.com/locate/regpep
The effects of reduced oxygen tension on swine granulosa cell
Giuseppina Basini a,*, Federico Bianco a, Francesca Grasselli a,
Martina Tirelli a, Simona Bussolati a, Carlo Tamanini b
a
Dipartimento di Produzioni Animali, Biotecnologie Veterinarie, Qualità e Sicurezza degli Alimenti-Sezione di Fisiologia Veterinaria,
Università di Parma, Via del Taglio 8, Parma 43100, Italy
b
DIMORFIPA, Università di Bologna, Via Tolara di Sopra 50, 40064 Ozzano Emilia, Bologna, Italy
Received 11 June 2003; received in revised form 10 February 2004; accepted 23 February 2004
Available online 25 March 2004
Abstract
Follicular growth is characterized by an augmented vascularization, possibly driven by a fall in the oxygen supply. The present study was
undertaken to investigate the effects of hypoxia on swine granulosa cells. At first, we quantified oxygen partial pressure ( pO2) in follicular
fluid from different size follicles; the granulosa cells collected from large follicles (>5 mm) were subjected for 18 h to normoxia (19% O2),
partial (5% O2) or total hypoxia (1% O2). The effects of these conditions were tested on the main parameters of granulosa cell function,
steroidogenesis and cell proliferation, and on vascular endothelial growth factor (VEGF), nitric oxide (NO) and superoxide anion (O2 )
production. Oxygen tension in follicular fluid was negatively related to follicular size, pointing out a gradual reduction during follicular
growth. Severe hypoxic conditions determined a reduction of both 17h estradiol and progesterone production, while partial hypoxia did not
seem to affect them. Hypoxia increased VEGF as well as O2 production in swine granulosa cells without impairing cell growth; in addition, it
decreased NO output.
We may conclude that physiological hypoxia could play a pivotal role in the follicular angiogenic process stimulating VEGF synthesis by
granulosa cells. ROS are possibly involved in hypoxic signalling.
D 2004 Elsevier B.V. All rights reserved.
Keywords: VEGF; Ovary; Nitric oxide; Superoxide anion; Steroid hormones
1. Introduction
The knowledge on angiogenesis, the process by which
new capillaries develop from preexisting vessels, has greatly
improved in the last years thanks to the research on cancer
[1]. Most of efforts have been addressed to the inhibition of
neovascularization in tumors, which always represents a
pathological process [2]. The only chance to study the
physiological pattern of the angiogenic process in the adult
is offered by the female reproductive system [3]. In particular, the ovary is distinctive since it represents a site of
active angiogenesis that takes place both in the growing
follicle and in the corpus luteum formation. The vascular
sheath that develops during follicular maturation in the
thecal compartment expands with ongoing folliculogenesis,
* Corresponding author. Tel.: +39-521-902775; fax: +39-521-902770.
E-mail address: basini@unipr.it (G. Basini).
0167-0115/$ - see front matter D 2004 Elsevier B.V. All rights reserved.
doi:10.1016/j.regpep.2004.02.013
but the thecal capillaries do not penetrate the membrana
propria; therefore, granulosa layer remains avascular until
breakdown of the basement membrane at ovulation [4,5].
The vasculature of the follicle is necessary for supplying
hormones and their precursors, oxygen and nutrients [6]; the
preferential delivery of gonadotropins via a more highly
developed vascular system in individual follicles has been
suggested to play an instrumental role in the selection and
growth of the dominant follicle [7]. It is worth noticing that
the increased thickness of the avascular granulosa layer
during follicular growth should result in a decrease of pO2
within the follicle, since these cells depend exclusively on
diffusion processes for nutrients and oxygen supply [8].
Extensive angiogenic responses in other tissues have been
shown to be elicited under circumstances in which oxygen
homeostasis is impaired [9].
Among the substances regulating the angiogenic process,
a key role is played by the vascular endothelial growth
70
G. Basini et al. / Regulatory Peptides 120 (2004) 69–75
factor (VEGF), also known as vascular permeability factor
(VPF), which is mitogen for endothelial cells and stimulates
vascular permeability [10 – 12].
The involvement of VEGF in follicular development is
supported by experimental data showing its increase in
follicular fluid during follicle growth [13] as well as a
positive relationship between VEGF production by granulosa cells and original follicular size [11,14].
Hypoxia has been shown to modulate VEGF production
[15] through the production of hypoxia-inducible factor
(HIF-1) [16], a transcription factor that functions as a master
regulator of oxygen homeostasis.
HIF-1 is not only regulated by oxygen tension, but also by
various other stimuli, among which it is worth remembering
nitric oxide (NO) [17]. Even though evidence exists on the
antiangiogenic properties of NO in the follicle [18], its involvement in hypoxia-mediated angiogenesis is not clear [19,20].
On this basis, we have undertaken the present study to
verify whether a relationship exists between hypoxia and
VEGF production within the ovarian follicle. To do this, we
quantified oxygen tension in swine follicles at different
stages of development; moreover, we tested the effects of
two hypoxic conditions on the production of VEGF, NO,
O2 and steroids as well as on proliferation of granulosa cells
collected from large follicles.
streptomycin (100 Ag/ml), amphotericin B (2.5 Ag/ml),
selenium (5 ng/ml) and transferrin (5 Ag/ml). Once seeded,
cells were incubated at 37 jC under humidified atmosphere
(5% CO2) for 24 h and then subjected for 18 h to normoxic
(19% O2), hypoxic (5% O2) or anoxic (1% O2) conditions.
Total hypoxia was achieved employing an AnaerocultR A
mini while partial hypoxia was obtained by means of an
AnaerocultR C mini (Merck, Darmstadt, Germany). In both
cases, the system consisted of plastic pouches and a paper
gas-generating sachet.
2.2. pO2 in follicular fluid
Follicular fluid was collected separately from individual
large and medium follicles containing enough fluid to fill a
cartridge (Samed, Merlino, Italy), while follicular fluid from
three small follicles was pooled in order to obtain a
sufficient amount. A total of 20 determinations for each
follicular class were carried out. Fluid was assayed for pO2
by means of an i-STAT R Portable Clinical Analyzer (iSTAT, Princeton, NJ, USA) [23] after ensuring quality
control with the electronic simulator as recommended by
the manufacturer. The integrity of the cartridges and the
calibration were verified before commencement of each
determination. The intra-assay coefficient of variation for
pO2 measurement was < 5%.
2. Materials and methods
2.3. Cell proliferation
All the reagents were obtained from Sigma (St. Louis,
MO, USA) unless otherwise specified.
Viable cells (104) were cultured in 200 Al CM at different
O2 tensions (as described above) and cell proliferation was
evaluated by 5-bromo-2V-deoxyuridine (BrdU) incorporation
assay test (Roche, Mannheim, Germany). Briefly, 20 Al BrdU
were added to each well during the last 4 h of incubation, then
culture media were removed and a DNA denaturating solution was added in order to improve the accessibility of the
incorporated BrdU for antibody detection. Thereafter, 100
Al anti-BrdU antibody were added to each well. After a 1.5
h incubation at 21 jC the immune complexes were detected
by the subsequent substrate reaction. The reaction product
was quantified by measuring the absorbance at 450 nm
against 690 nm using a Spectra Shell Microplate reader
(SLT Spectra, Milan, Italy). To establish viable cell number,
absorbance was related to a standard curve prepared by
culturing in quintuplicate granulosa cells at different plating
densities (from 103 to 105/200 Al) for 48 h. The curve was
repeated in four different experiments. The relationship
between cell number and absorbance resulted linear
(r = 0.92). Cell number/well was estimated from the resulting
linear regression equation. The assay detection limit was 103
cells/well and the variation coefficient was less than 5%.
2.1. Follicular fluid and granulosa cell collection
Swine ovaries were collected at a local slaughterhouse,
placed into cold PBS (4 jC) supplemented with penicillin
(500 IU/ml), streptomycin (500 Ag/ml) and amphotericin B
(3.75 Ag/ml), maintained in a freezer bag and transported to
the laboratory within 1 h. After a series of washing with
PBS and ethanol (70%) follicles were divided into three
classes corresponding to the diameter: small ( < 3mm),
medium (3– 5 mm) and large follicles (>5 mm). Follicular
fluid was collected with a 26-gauge needle from follicles of
each class to determine the O2 tension.
Granulosa cells from large follicles were aseptically harvested by aspiration with a 26-gauge needle and released in
medium containg heparin (50 IU/ml), centrifuged for pelleting and then treated with 0.9% prewarmed ammonium
chloride at 37 jC for 1 min to remove red blood cells. Cell
number and viability were estimated using a haemocytometer
under a phase contrast microscope after vital staining with
trypan blue (0.4%) of an aliquot of the cell suspension. Cells
were seeded at different plating densities (see below) in
serum-free culture medium (CM) [21,22] composed by
M199 supplemented with sodium bicarbonate (2.2 mg/ml),
bovine serum albumin (BSA 0.1%), penicillin (100 IU/ml),
2.4. WST-1 assay for superoxide (O2 ) production
O2 production was evaluated by the cell proliferation
WST-1 test (Roche) applied to the same culture protocol
71
G. Basini et al. / Regulatory Peptides 120 (2004) 69–75
Fig. 1. pO2 levels in swine follicular fluid. Data are expressed as
mean F S.E.M. Different letters indicate a significant difference ( p < 0.05).
used above, since evidence also exists that tetrazolium salts
can be used as a reliable measure of intracellular O2
production [24,25]. Briefly, 20 Al WST-1 were added to
the cells during the last 4 h of incubation and absorbance
was then determined using a Spectra Shell Microplate reader
at 450 nm against 620 nm.
2.5. VEGF production
Cells (106) in 1 ml CM + 1% FCS were seeded in 24-well
plates and incubated for 48 h. VEGF content in culture
media was quantified by an ELISA (Quantikine, R&D
System, Minneapolis, MN, USA); this assay, developed
for human VEGF detection, has been validated for pig
VEGF [26]. The assay sensitivity was 0.23 pmol/l, the
inter- and intra-assay CVs were always less than 7%. A
Spectra Shell microplate reader, set to read 450 nm emission, was used to quantify the reaction product.
2.6. NO production
A total of 105 cells/200 Al CM were seeded in 96well plates and incubated in the conditions described
Fig. 3. Effect of partial and total hypoxia on O2 generation by 104 swine
granulosa cells. Data are expressed as mean F S.E.M. Different letters
indicate a significant difference ( p < 0.05).
above. NO was assessed by measuring nitrite levels in
culture media by the microplate method based on the
formation of chromophore after reaction with Greiss
reagent, which was prepared fresh daily by mixing equal
volumes of stock A (1% sulfanilamide, 5% phosphoric
acid) and stock B (0.1% N-[naphthyl] ethylenediamine
dihydrochloride) [27].
2.7. Steroid production
A total of 104 cells/well were seeded in 96-well plates in
200 Al CM supplemented with androstenedione (28 ng/ml).
Culture media were then collected, frozen and stored at 20
jC until progesterone (P4) and 17h estradiol (E2) determination by validated RIAs [28].
P4 assay sensitivity and ED50 were 0.24 and 1 nmol/l,
respectively; E2 assay sensitivity and ED50 were 0.05 and
0.2 nmol/l. The intra- and inter-assay coefficients of variation were less than 12% for both assays.
2.8. Statistical analysis
Each experiment was repeated at least four times (six
replicates per treatment). Experimental data are presented
as mean F S.E.M.; statistical differences between treatments were calculated with ANOVA using Statgraphics
package (STSC, Rockville, MD, USA). When significant
differences were found, means were compared by
Scheffè’s F-test.
Table 1
Effect of partial and total hypoxia on VEGF and NO production by 106 and
105 swine granulosa cells, respectively
VEGF (pg/ml)
NO (AM)
Fig. 2. Effect of partial and total hypoxia on swine granulosa cells number.
Data are expressed as mean F S.E.M.
Control
Partial hypoxia
Total hypoxia
1061 F 90 a
3.16 F 0.3 a
2333 F 179.6 b
1.93 F 0.2 b
2729 F 107.1 b
1.47 F 0.1 b
Data are expressed as mean F S.E.M. Different letters indicate a significant
difference ( p < 0.05).
72
G. Basini et al. / Regulatory Peptides 120 (2004) 69–75
3. Results
3.4. VEGF production
3.1. pO2 in follicular fluid
VEGF concentrations in control group (1061 F 90 pg/
ml) were significantly ( p < 0.05) increased by both partial
and total hypoxia (Table 1); no differences were observed
between these two conditions.
pO2 levels were 126.9 F 2 mm Hg (means F S.E.M.) in
small follicles and decreased to 93.4 F 3 and 67.7 F 2 mm
Hg in medium and large follicles respectively (Fig. 1); the
differences between the three follicular classes were significant ( p < 0.05).
3.2. Cell proliferation
BrdU incorporation assay did not evidence any significant effect of hypoxia on cell proliferation: in fact, a fivefold
increase in cell number was observed both in normoxia and
hypoxia (Fig. 2).
3.3. O2 production
Hypoxia significantly stimulated ( p < 0.05) O2 generation: both total and partial hypoxic conditions exerted
similar effects (Fig. 3).
3.5. NO production
In the control group, NO levels were 3.16 F 0.33 AM; a
marked decrease was observed both in total and partial
hypoxia ( p < 0.05) with no significant differences between
the two hypoxic conditions (Table 1).
3.6. Steroid production
E2 and P4 levels in the control group were 5.5 F 0.5 and
84.7 F 8.9 ng/ml, respectively.
Both E2 and P4 levels were significantly ( p < 0.05)
reduced in total hypoxia (Fig. 4), while no significant effect
was observed under partial hypoxic condition.
4. Discussion
Fig. 4. Effect of partial and total hypoxia on E2 (a) and P4 (b)
production by 104 swine granulosa cells. Data are expressed as
mean F S.E.M. Different letters indicate a significant difference
( p < 0.05).
Several authors [29 – 31] evidenced that a sustained
increase in oxygen consumption or a functional impairment
of existing vasculature, both resulting in insufficient perfusion, triggers neovascularization. On this basis, our first goal
was to measure oxygen partial pressure ( pO2) in follicular
fluid which resulted negatively related to follicular size, in
accordance with the observations by Fischer et al. [4].
It has long been recognized that tissues respond to
ischemia by producing angiogenic factors that recruit
new blood vessels to the ischemic area. However, despite
considerable progress has been made in the understanding
of the pathways which are activated during cellular hypoxia, no consensus has been reached on the mechanism by
which O2 sensing is achieved [32,33]. Since the mitochondrion is the major oxygen-consuming organelle, it might
be expected to play a central role in oxygen-sensitive
processes by varying the production of reactive oxygen
species (ROS) during hypoxia [34,35]. There is a growing
consensus that the cellular O2 sensors are redox-based.
Among the variety of possible molecular sensors, NADH
oxidase and NADPH oxidase have been indicated as the
most important [36,37], presumably as a result of the
increased availability of NADH during hypoxia. Several
studies [38,39] indicate that the response involves an
increase of superoxide (O2 ) production by NADH and
NADPH oxidase.
Tetrazolium salts are widely used to measure cell
proliferation and viability. Their function has been shown
to depend on cellular production of reduced pyridine
nucleotides: these cofactors act as substrates for cellular
oxidoreductases that reduce tetrazolium salts (such as
G. Basini et al. / Regulatory Peptides 120 (2004) 69–75
MTT, XTT, MTS and, more recently, WST-1) to formazan
end-products [40].
Our data on WST-1 reduction suggest that low oxygen
may cause an increase of O2 production in granulosa cells
without affecting cell proliferation, as indicated by thymidine uptake.
Cells subjected to hypoxic environment have been demonstrated to exhibit a variety of biological responses,
including the activation of signalling pathways that regulate
proliferation [41]. To our knowledge, the effect of hypoxia
on granulosa cell proliferation has never been examined;
hypoxia has been found to exert a stimulatory effect on the
growth of both endothelial cells from human umbilical vein
[42] and neurons [43] and to inhibit osteoblasts [44] and
bone marrow cell proliferation [45]; the reasons for these
discrepancies are unclear, but the response likely depends
on the cell type.
Yoshino et al. [46] demonstrated that hypoxia is a major
inducer of angiogenic factors such as interleukin-8 and
VEGF, a peptide described both as a specific mitogen for
vascular endothelial cells and as a factor that increases
vascular permeability [47,48]. Wang et al. [49] reported
that hypoxia-induced transcription of VEGF mRNA
involves a specific transcription factor known as hypoxiainducible factor (HIF).
In a previous work [14] we showed that porcine
granulosa cells represent a site of VEGF production which
appears to be maximal in cells from large follicles. The
present observations suggest that hypoxia can be responsible for these high levels. In fact, the increase in follicular
diameter during maturation is accompanied by a decreased
oxygen tension in follicular fluid which appears to negatively affect VEGF production by granulosa cells. Collectively, these results point out the important role of hypoxia
in the development of an extensive vascular network
driven by VEGF within the follicle wall; nevertheless,
others [50] reported conflicting data, which do not support
a model for hypoxic stress promoting VEGF production by
granulosa cells.
By the way, hypoxia is not the only factor that regulates
VEGF production. Nitric oxide (NO), a highly diffusible gas
synthesized by NO synthases (NOS) from L-arginine and
molecular O2, has been recognized as a positive or negative
modulator of VEGF synthesis [51]. In a previous work [18],
we showed that the treatment with S-nitroso-L-acetyl penicillamine (SNAP), a potent NO donor, reduces VEGF
production by granulosa cells, thus suggesting that NO
may play an anti-angiogenic role within the ovary; a
negative loop between VEGF and NO is also confirmed
by the finding that VEGF inhibits NO production by
granulosa cells [14]. Several studies have examined the
regulation of NOS activity by O2 tension in cultured cells:
McCormick et al. [52] found that although hypoxia
increases inducible NOS gene expression in macrophages,
NO synthesis is markedly reduced. Whorton et al. [53]
demonstrated that exposure to hypoxia reduces NO produc-
73
tion by endothelial NOS. Our results are in agreement with
those of Steiner et al. [54] who showed that hypoxia results
in oxidative stress due to a change in the ROS –NO balance.
However, the mechanisms underlying these changes are
unclear. Two alternative explanations are possible: (1)
excess ROS generated during hypoxia consume NO, since
it acts as an antioxidant; (2) the reduced availability of O2
substrate negatively affect NOS, thus decreasing NO production and increasing in the meanwhile ROS levels.
Further studies are needed in order to clarify this important
point.
The adaptation to hypoxia involves an integrated response among different cell functions [55]. The effect of
reduced oxygen tension on ovarian steroidogenesis has been
examined by Koos and Feiertag [56] who demonstrated that
hypoxia inhibits P4 accumulation in rat granulosa cell
culture. Low oxygen tension has been demonstrated to
prevent E2 secretion in ED27 cells [57], P4 production by
placental villous cells [58] and P4 and E2 synthesis in
isolated trophoblast in culture [59]. Our results show that
both P4 and E2 production are reduced in total but not in
partial hypoxia as recently reported by Martinez-Chequer et
al. [50]. It is worth noticing that a severe hypoxic milieu is
not representative of the in vivo situation, as confirmed by
our present data about pO2 tension in follicular fluid; partial
hypoxic conditions are possibly more comparable to those
characterizing the well developed ovarian follicle, which
relies on E2 and P4 production for its survival [60]. Severe
hypoxia has been suggested to inhibit P450 side chain
cleavage [61], for which O2 represents an essential co-factor
in different cell types [62,63].
We may argue that ROS could play some role in inhibiting
steroidogenesis: low oxygen tension appears to increase ROS
generation [64], which have been demonstrated to exert
antisteroidogenic effect in granulosa cells [65,66].
Taken together, our current data suggest that large swine
follicles are physiologically exposed to oxygen shortage.
This condition would activate a mechanism which, via
VEGF, ensures a proper blood supply to the growing
follicle. ROS likely play a crucial role in mediating hypoxic
signal. The reduction of O2 milieu, if not maximal, does not
seem to impair steroid production by granulosa cells.
Acknowledgements
This research was supported by a MIUR COFIN grant.
References
[1] Teo NB, Shoker BS, Martin L, Sloane JP, Holcombe C. Angiogenesis
in pre-invasive cancers. Anticancer Res 2002;22:2061 – 72.
[2] Folkman J. Role of angiogenesis in tumor growth and metastasis.
Semin Oncol 2002;29:15 – 8.
[3] Fraser HM, Lunn SF. Angiogenesis and its control in the female
reproductive system. Br Med Bull 2000;56:787 – 97.
74
G. Basini et al. / Regulatory Peptides 120 (2004) 69–75
[4] Fischer B, Kunzel W, Kleinstein J, Gips H. Oxygen tension in follicular fluid falls with follicle maturation. Eur J Obstet Gynecol Reprod
Biol 1992;43:39 – 43.
[5] Reynolds LP, Grazul-Bilska AT, Redmer DA. Angiogenesis in the
female reproductive organs: pathological implications. Int J Exp
Pathol 2002;83:151 – 63.
[6] Neeman M, Abramovitch R, Schiffenbauer YS, Tempel C. Regulation
of angiogenesis by hypoxic stress: from solid tumours to the ovarian
follicle. Int J Exp Pathol 1997;78:57 – 70.
[7] Wulff C, Wiegand SJ, Saunders PT, Scobie GA, Fraser HM. Angiogenesis during follicular development in the primate and its inhibition
by treatment with truncated Flt-1-Fc (vascular endothelial growth
factor TrapA40). Endocrinology 2001;142:3244 – 54.
[8] Van Blerkom J, Antczak M, Schrader R. The developmental potential
of the human oocyte is related to the dissolved oxygen content of
follicular fluid: association with vascular endothelial growth factor
levels and perifollicular blood flow characteristics. Hum Reprod
1997;12:1047 – 55.
[9] Dor V, Di Donato M, Sabatier M, Montiglio F, Civaia F. Left ventricular
reconstruction by endoventricular circular patch plasty repair: a 17-year
experience. Semin Thorac Cardiovasc Surg 2001;13:435 – 47.
[10] Frelin C, Ladoux A, Dangelo G. Vascular endothelial growth factors
and angiogenesis. Ann Endocrinol (Paris) 2000;61:70 – 4.
[11] Geva E, Jaffe RB. Role of vascular endothelial growth factor in
ovarian physiology and pathology. Fertil Steril 2000;74:429 – 38.
[12] Ferrara N. Role of vascular endothelial growth factor in physiologic
and pathologic angiogenesis: therapeutic implications. Semin Oncol
2002;29:10 – 4.
[13] Mattioli M, Barboni B, Turriani M, Galeati G, Zannoni A, Castellani
G, et al. Follicle activation involves vascular endothelial growth factor
production and increased blood vessel extension. Biol Reprod 2001;
65:1014 – 9.
[14] Grasselli F, Basini G, Bussolati S, Tamanini C. Effects of VEGF and
bFGF on proliferation and production of steroids and nitric oxide in
porcine granulosa cells. Reprod Domest Anim 2002;37:362 – 8.
[15] Sharkey AM, Day K, McPherson A, Malik S, Licence D, Smith SK,
et al. Vascular endothelial growth factor expression in human endometrium is regulated by hypoxia. J Clin Endocrinol Metab 2000;
85:402 – 9.
[16] Horiuchi A, Imai T, Shimizu M, Oka K, Wang C, Nikaido T, et al.
Hypoxia-induced changes in the expression of VEGF, HIF-1 alpha
and cell cycle-related molecules in ovarian cancer cells. Anticancer
Res 2002;22:2697 – 702.
[17] Chun YS, Kim MS, Park JW. Oxygen-dependent and -independent
regulation of HIF-1alpha. J Korean Med Sci 2002;17:581 – 8.
[18] Grasselli, F., Basini, G., Cavalli, V., Tirelli, M., Tamanini, C., Nitric
oxide inhibits VEGF production by cultured swine granulosa cells.
Vienna, AU: ESDAR; 2001. Abstract 60.
[19] Ziche M, Morbidelli L. Determination of angiogenesis-regulating
properties of NO. Methods Enzymol 2002;352:407 – 21.
[20] Agani FH, Puchowicz M, Chavez JC, Pichiule P, LaManna J. Role of
nitric oxide in the regulation of HIF-1a expression during hypoxia.
Am J Physiol, Cell Physiol 2002;283:178 – 86.
[21] Basini G, Tamanini C. Selenium stimulates estradiol production in
bovine granulosa cells: possible involvement of nitric oxide. Domest
Anim Endocrinol 2000;18:1 – 17.
[22] Grasselli F, Ponderato N, Basini G, Tamanini C. Nitric oxide synthase
expression and nitric oxide/cyclic GMP pathway in swine granulosa
cells. Domest Anim Endocrinol 2001;20:241 – 52.
[23] Huey S, Abuhamad A, Barroso G, Hsu MI, Kolm P, Mayer J, et al.
Perifollicular blood flow Doppler indices, but not follicular pO2,
pCO2, or pH, predict oocyte developmental competence in vitro fertilization. Fertil Steril 1999;72:707 – 12.
[24] Benov L, Fridovich I. Is reduction of the sulfonated tetrazolium 2,3bis (2-methoxy-4-nitro-5-sulfophenyl)-2-tetrazolium 5-carboxanilide
a reliable measure of intracellular superoxide production? Anal Biochem 2002;310:186 – 90.
[25] Ukeda H, Shimamura T, Tsubouchi M, Harada Y, Nakai Y, Sawamura
M. Spectrophotometric assay of superoxide anion formed in Maillard
reaction based on highly water-soluble tetrazolium salt. Anal Sci
2002;18:1151 – 4.
[26] Barboni B, Turriani M, Galeati G, Spinaci M, Bacci ML, Forni M, et al.
Vascular endothelial growth factor production in growing pig antral
follicles. Biol Reprod 2000;63:858 – 64.
[27] Dong YL, Yallampalli C. Interaction between nitric oxide and prostaglandin E2 pathways in pregnant rat uteri. Am J Physiol 1996;270:
471 – 6.
[28] Grasselli F, Baratta M, Tamanini C. Effects of a GnRH analogue
(buserelin) infused via osmotic minipumps on pituitary and ovarian
activity of prepuberal heifers. Anim Reprod Sci 1993;32:153 – 61.
[29] Sipos B, Weber D, Ungefroren H, Kalthoff H, Zuhlsdorff A, Luther C,
et al. Vascular endothelial growth factor mediated angiogenic potential of pancreatic ductal carcinomas enhanced by hypoxia: an in vitro
and in vivo study. Int J Cancer 2002;102:592 – 600.
[30] Chiarug V, Ruggiero M, Magnelli L. Angiogenesis and the unique
nature of tumor matrix. Mol Biotechnol 2002;21:85 – 90.
[31] Iida T, Yannuzzi LA, Freund KB, Ciardella AP, Costa DL, Huang SJ,
et al. Retinal angiopathy and polypoidal choroidal vasculopathy. Retina 2002;22:455 – 63.
[32] Chandel NS, Schumacker PT. Cellular oxygen sensing by mitochondria: old questions, new insight. J Appl Physiol 2000;88:1880 – 9.
[33] Maxwell PH, Ratcliffe PJ. Oxygen sensors and angiogenesis. Semin
Cell Dev Biol 2002;13:29 – 37.
[34] Maulik N, Das DK. Redox signaling in vascular angiogenesis. Free
Radic Biol Med 2002;33:1047 – 60.
[35] Kulisz A, Chen N, Chandel NS, Shao Z, Schumacker PT. Mitochondrial ROS initiate phosphorylation of p38 MAP kinase during hypoxia in cardiomyocytes. Am J Physiol, Lung Cell Mol Physiol 2002;
282:1324 – 9.
[36] Mohazzab-H KM, Agarwal R, Wolin MS. Influence of glutathione
peroxidase on coronary artery responses to alterations in PO2 and
H2O2. Am J Physiol 1999;276:235 – 41.
[37] Michelakis ED, Hampl V, Nsair A, Wu X, Harry G, Haromy A, et al.
Diversity in mitochondrial function explains differences in vascular
oxygen sensing. Circ Res 2002;90:1307 – 15.
[38] Lopez-Barneo J, Pardal R, Ortega-Saenz P. Cellular mechanism of
oxygen sensing. Annu Rev Physiol 2001;63:259 – 87.
[39] Gonzalez C, Sanz-Alfayate G, Agapito MT, Gomez-Nino A, Rocher
A, Obeso A. Significance of ROS in oxygen sensing in cell systems
with sensitivity to physiological hypoxia. Respir Physiol, Neurobiol
2002;132:17 – 41.
[40] Tan AS, Berridge MV. Superoxide produced by activated neutrophils
efficiently reduces the tetrazolium salt, WST-1 to produce a soluble
formazan: a simple colorimetric assay for measuring respiratory burst
activation and for screening anti-inflammatory agents. J Immunol
Methods 2000;238:59 – 68.
[41] Harris AL. Hypoxia a key regulatory factor in tumour growth. Nat
Rev, Cancer 2002;2:38 – 47.
[42] Bednarek W, Czekierdowski A, Kraczkowski J, Kotarski J. The influence of hypoxia on the proliferation of endothelial cells originating
from human umbilical vein (HUVEC): an in vitro study. Ginekol Pol
2001;72:1567 – 71.
[43] Studer L, Csete M, Lee SH, Kabbani N, Walikonis J, Wold B, et al.
Enhanced proliferation, survival, and dopaminergic differentiation of
CNS precursors in lowered oxygen. J Neurosci 2000;20:7377 – 83.
[44] Steinbrech DS, Mehrara BJ, Saadeh PB, Chin G, Dudziak ME,
Gerrets RP, et al. Hypoxia regulates VEGF expression and cellular
proliferation by osteoblasts in vitro. Plast Reconstr Surg 1999;104:
738 – 47.
[45] Jensen PO, Mortensen BT, Hodgkiss RJ, Iversen PO, Christensen IJ,
Helledie N, et al. Increased cellular hypoxia and reduced proliferation
of both normal and leukaemic cells during progression of acute myeloid leukaemia in rats. Cell Prolif 2000;33:381 – 95.
[46] Yoshino O, Osuga Y, Koga K, Hirota Y, Yano T, Tsutsumi O, et al.
G. Basini et al. / Regulatory Peptides 120 (2004) 69–75
[47]
[48]
[49]
[50]
[51]
[52]
[53]
[54]
[55]
[56]
Upregulation of interleukin-8 by hypoxia in human ovaries. Am J
Reprod Immunol 2003;50:286 – 90.
Leung DW, Cachianes G, Kuang WJ, Goeddel DV, Ferrara N. Vascular endothelial growth factor is a secreted angiogenic mitogen.
Science 1989;246:1306 – 9.
Shweiki D, Itin A, Soffer D, Keshet E. Vascular endothelial growth
factor induced by hypoxia may mediate hypoxia-initiated angiogenesis. Nature 1992;359:843 – 5.
Wang GL, Jiang BH, Rue EA, Semenza GL. Hypoxia-inducible factor
1 is a basic-helix-loop-helix-PAS heterodimer regulated by cellular O2
tension. Proc Natl Acad Sci 1995;92:5510 – 4.
Martinez-Chequer JC, Stouffer RL, Hazzard TM, Patton PE, Molskness TA. Insulin-like growth factors-1 and -2, but not hypoxia, synergize with gonadotropin hormone to promote vascular endothelial
growth factor-A secretion by monkey granulosa cells from preovulatory follicles. Biol Reprod 2003;68:1112 – 8.
Dulak J, Jozkowicz A. Regulation of vascular endothelial growth
factor synthesis by nitric oxide: facts and controversies. Antioxid
Redox Signal 2003;5:123 – 32.
McCormick CC, Li WP, Calero M. Oxygen tension limits nitric oxide
synthesis by activated macrophages. Biochem J 2000;350:709 – 16.
Whorton AR, Simonds DB, Piantadosi CA. Regulation of nitric oxide
synthesis by oxygen in vascular endothelial cells. Am J Physiol
1997;272:1161 – 6.
Steiner DR, Gonzalez NC, Wood JG. Interaction between reactive
oxygen species and nitric oxide in the microvascular response to
systemic hypoxia. J Appl Physiol 2002;93:1411 – 8.
Boutilier RG. Mechanisms of cell survival in hypoxia and hypothermia. J Exp Biol 2001;204:3171 – 81.
Koos RD, Feiertag MA. The effect of reduced oxygen tension on
[57]
[58]
[59]
[60]
[61]
[62]
[63]
[64]
[65]
[66]
75
progesterone accumulation in rat granulosa cell cultures. Steroids
1989;54:553 – 62.
Ma T, Yang ST, Kniss DA. Oxygen tension influences proliferation
and differentiation in a tissue-engineered model of placental trophoblast-like cells. Tissue Eng 2001;7:495 – 506.
Kay HH, Robinette B, Shin YY, Siew P, Shellhaas CS, Tyrey L.
Placental villous glucose metabolism and hormone release respond
to varying oxygen tensions. J Soc Gynecol Investig 1997;4:241 – 6.
Esterman A, Finlay TH, Dancis J. The effect of hypoxia on term
trophoblast: hormone synthesis and release. Placenta 1996;17:
217 – 22.
Hillier SG. Gonadotropic control of ovarian follicular growth and
development. Mol Cell Endocrinol 2001;179:39 – 46.
Lieberman S, Lin YY. Reflections on sterol sidechain cleavage process catalyzed by cytochrome P450(scc). J Steroid Biochem Mol Biol
2001;78:1 – 14.
Bruder ED, Nagler AK, Raff H. Oxygen-dependence of ACTH-stimulated aldosterone and corticosterone synthesis in the rat adrenal cortex: developmental aspects. J Endocrinol 2002;172:595 – 604.
Raff H, Jankowski B. O2 dependence of pregnenolone and aldosterone synthesis in mitochondria from bovine zona glomerulosa cells. J
Appl Physiol 1995;78:1625 – 8.
Maulik N. Redox signaling of angiogenesis. Antioxid Redox Signal
2002;4:805 – 15.
Margolin Y, Aten RF, Behrman HR. Antigonadotropic and antisteroidogenic actions of peroxide in rat granulosa cells. Endocrinology
1990;127:245 – 50.
Behrman HR, Kodaman PH, Preston SL, Gao S. Oxidative stress and
the ovary. J Soc Gynecol Investig 2001;8:40 – 2.