Upload
others
View
1
Download
0
Embed Size (px)
Citation preview
1 Thorey et al.
Transgenic mice reveal novel activities of growth hormone
in wound repair, angiogenesis and myofibroblast
differentiation
Irmgard S. Thorey1,2, Boris Hinz3, Andreas Hoeflich2, Susanne
Kaesler1, Philippe Bugnon1, Martin Elmlinger4, Rüdiger Wanke5,
Eckhard Wolf2 and Sabine Werner1
1Institute of Cell Biology, Department of Biology, ETH Zürich, Hönggerberg,
CH-8093 Zürich, Switzerland 2Institute of Molecular Animal Breeding/Gene Center, Ludwig-Maximilians-
University, Feodor-Lynen-Str. 25, D-81377 Munich, Germany 3Laboratory of Cell Biophysics, Swiss Federal Institute of Technology (EPFL),
Bâtiment SG - AA-B 143, CH-1015 Lausanne, Switzerland 4Pediatric Endocrinology, Children’s Hospital, University of Tübingen,
D-72076 Tübingen, Germany 5Institute of Veterinary Pathology, Ludwig-Maximilians-University, Munich,
Germany
Address for correspondence:
Dr. Sabine Werner Institute of Cell Biology
ETH Zürich, Hönggerberg, CH-8093 Zürich, Switzerland
Phone: 41-1-633-3941 Fax: 41-1-633-1174
E-mail: [email protected]
Running title: Growth hormone and wound healing
JBC Papers in Press. Published on April 7, 2004 as Manuscript M311467200
Copyright 2004 by The American Society for Biochemistry and Molecular Biology, Inc.
by guest on August 17, 2020
http://ww
w.jbc.org/
Dow
nloaded from
2 Thorey et al.
Abstract
An increasing number of patients is being treated with growth hormone (GH)
for the enhancement of body growth, but also as an anti-aging strategy.
However, the side effects of GH have been poorly defined. In this study we
determined the effect of GH on wound repair and its mechanisms of action at
the wound site. For this purpose, we performed wound healing studies in
transgenic mice overexpressing GH. Full-thickness incisional and excisional
wounds of transgenic animals developed an extensive, highly vascularized
granulation tissue. However, wound bursting strength was not increased.
Wound closure was strongly delayed as a result of enhanced granulation
tissue formation and impaired wound contraction. The latter effect is most
likely due to a significantly reduced number of myofibroblasts at the wound
site. Using in vitro studies with stressed collagen lattices, we identified GH as
an inhibitor of transforming growth factor β-induced myofibroblast
differentiation, resulting in a reduction in fibroblast contractile activity. These
results reveal novel roles of growth hormone in angiogenesis and
myofibroblast differentiation, which are most likely not mediated via insulin-
like growth factors at the wound site. Furthermore, our data suggest that
systemic GH treatment is detrimental for wound healing in non-healing
impaired individuals.
by guest on August 17, 2020
http://ww
w.jbc.org/
Dow
nloaded from
3 Thorey et al.
Introduction
Injury to the skin initiates a series of events, which finally lead to at least
partial reconstruction of the wounded tissue (1). The important role of locally
acting cytokines and growth factors in wound repair is well documented (2).
However, crucial functions of endocrine acting hormones have only recently
been recognized (3-5). One of the hormones, which are thought to influence
the repair process, is growth hormone (GH). This hormone is successfully
used for the treatment of growth defects in children. In addition, an increasing
number of healthy adult patients receive GH therapy as an anti-aging strategy
(6). However, the side effects of GH treatment have been poorly defined and
it is as yet unclear if GH affects the wound healing process in healthy
individuals.
Treatment with recombinant GH has been used in patients with severe burn
injuries, and in most studies enhanced rates of wound healing and patient
survival were observed (7). In addition, GH was shown to stimulate
granulation tissue formation and biomechanical wound strength in animal
models of impaired healing (8-11), although a lack of efficacy of GH has also
been reported (12, 13). Thus, the role of GH in wound repair remains to be
determined. In particular, the mechanisms of GH action in this process have
not yet been elucidated.
Many effects of GH are mediated via the insulin-like growth factor (IGF)
system (14), suggesting that this might also be a mechanism of GH action in
the skin. IGF-I is a mitogen for keratinocytes (15), and it stimulates collagen,
glycosaminoglycane and proteoglycane synthesis by dermal fibroblasts (16,
17). It exerts its effects in concert with a family of six IGF-binding proteins
(IGFBPs) which control the availability of IGF for signaling through its receptor
in a complex manner: While IGFBP-3 and IGFBP-4 have a predominantly
negative effect on IGF activity, IGFBP-5 can act to enhance IGF signaling, but
only when associated with the surface extracellular matrix of target cells (16,
by guest on August 17, 2020
http://ww
w.jbc.org/
Dow
nloaded from
4 Thorey et al.
18). In addition, IGFBPs have also IGF-independent effects on cell growth
(19).
Interestingly, imbalances in the IGF/IGFBP system are associated with wound
healing abnormalities. Thus, up-regulation of IGF or IGFBPs was detected in
hypertrophic scars, while decreased IGF levels were found in diabetic skin
and foot ulcers, and in the wounds of healing-impaired diabetic or
glucocorticoid-treated rats or mice (2). Based on these findings, the effect of
members of the IGF system on dermal tissue repair has been analyzed: Local
IGF gene therapy or protein treatment improved the wound healing process in
different animal models (20-23). In contrast, raising the serum levels of IGF-I
by systemic application did not improve wound healing, whereas GH was
effective in the same experimental set-up, possibly via induction of IGF-I at
the wound site (24).
These findings, together with the obvious importance of the GH/IGF system in
the homeostasis of the skin, prompted us to analyze the wound healing
process in transgenic mice overexpressing bovine GH (bGH) under a
phosphoenolpyruvate carboxykinase (PEPCK) promoter. These mice have
greatly elevated postnatal serum GH levels of ca. 2000 ng/ml (compared to
less than 10 ng/ml endogenous hormone in control mice), and serum IGF-I
levels which are 2-3 times higher than those of control littermates. In contrast
to growth hormone treatment models, these animals allow long-term studies
without immunologic complications (25). Interestingly, the skin of these
animals has a significantly increased absolute (males and females) and
relative weight (males only) (26, 27). GH transgenic males develop a
phenotype, which has been likened to an “oversized coat”. While skin
alterations in females are moderate, males develop a pronounced dermal
hypertrophy with dermal fibrosis and decreased subcutaneous adipose
by guest on August 17, 2020
http://ww
w.jbc.org/
Dow
nloaded from
5 Thorey et al.
tissue. This male-specific phenotype is dependent on androgen production
(26). Here we show that both transgenic males and females suffer from
severe wound healing abnormalities.
by guest on August 17, 2020
http://ww
w.jbc.org/
Dow
nloaded from
6 Thorey et al.
Experimental Procedures
Animals, wounding and preparation of wound tissue. Hemizygous
PEPCK-bGH transgenic mice in an NMRI outbred background were bred with
C57BL/6 wild-type mice. Transgenic and non-transgenic littermates were
anaesthetised by intraperitoneal (i.p.) injection of ketamine (10 g/l)/xylazine (8
g/l) solution (250µl/25g body weight). Four full-thickness excisional wounds, 5
mm diameter each, were made on either side of the dorsal midline by
excising skin and panniculus carnosus. Wounds were left uncovered and
harvested 5 or 13 days after injury. Mice were housed individually during the
healing period. For expression analyses, two complete wounds from each
animal including 2 mm of the epithelial margins were excised and immediately
frozen in liquid nitrogen. Non-wounded back skin served as a control. For
histological analysis the complete wounds were isolated, bisected, fixed
overnight in 4% paraformaldehyde in PBS (for histology) or 95% ethanol/1%
acetic acid (for immunofluorescence, bromodeoxyuridine (BrdU) staining and
morphometry) and embedded in paraffin. Sections (7 µm) from the middle of
the wound were stained using the Masson Trichrome procedure.
Morphometrical measurements of area and length were performed on BrdU-
stained sections using the OpenLab software (Improvision Ltd., Basel,
Switzerland) and are represented as single data points and median.
Alternatively, all values ranging from 25% below and above the median were
represented as boxes (25th tp 75th percentile). In this case the highest and
lowest values were also indicated as bars. Statistical significance of
differences was determined by the Mann-Whitney U test for non-Gaussian
distribution. All experiments with animals were carried out with permission
from the local veterinary authorities.
Wound bursting strength. Mice were anesthetized as described above. The
by guest on August 17, 2020
http://ww
w.jbc.org/
Dow
nloaded from
7 Thorey et al.
dorsal region was shaved and treated with a depilatory agent (Pilca Perfect,
Stafford-Miller Continental, Oevel, Belgium). Two full-thickness incisions (1
cm) were made at one anterior and one posterior, dorsal site, and the skin
margins were closed with strips of a wound plaster (Fixomull stretch,
Beiersdorf, Hamburg, Germany). Mice were sacrificed on day 5 post-
wounding, and bursting strength of the wounds was determined in situ using
the BTC-2000 system (SRLI Technologies, Nashville, TN) according to the
manufacturer`s protocol for the non-human disruptive linear incision analysis.
Data are shown as median, 25th to 75th percentile, and highest and lowest
value. Statistical significance of differences in tensile strength between the
groups was determined by the Mann-Whitney U test.
Labelling with bromodeoxyuridine (BrdU). BrdU labelling was performed
as described (28). Sections (7 µm) from the middle of the wound were
incubated with a peroxidase-conjugated monoclonal antibody directed against
BrdU (Roche Diagnostics Ltd, Rotkreuz, Switzerland) and stained with 0.05%
diaminobenzidine/0.01% H2O2.
Immunofluorescence and immunohistochemistry. Acetic acid/ethanol-
fixed paraffin sections (7 µm) from the middle of the wound or immortalized
mouse embryonic fibroblasts were incubated with antibodies directed against
α-smooth muscle actin (SMA) (anti-αSM-1, IgG2a mAb (28)), ED-A
fibronectin (IST-9, IgG1 mAb, kind gift from Dr. L. Zardi, National Institute for
Cancer Research, Laboratory of Cell Biology, Genova, Italy (29)), desmin
(D33, IgG1 mAb, Dako, Copenhagen, Denmark), PECAM-1 (BD Biosciences,
Heidelberg, Germany), Ly-6G (BD Biosciences), F4/80 (Serotec, Oxford, UK),
cytokeratins 6, 14 (Babco, Richmond, CA) and 10 (Dako), followed by Cy2-,
Cy3-, Cy5-, FITC- or TRITC-, Alexa647- or Alexa568-conjugated conjugated
secondary antibodies (Jackson Immunoresearch Laboratory Inc., West
by guest on August 17, 2020
http://ww
w.jbc.org/
Dow
nloaded from
8 Thorey et al.
Grove, PA, USA and Molecular Probes, Eugene, OR). Cell nuclei were
stained with DAPI (Sigma, Munich, Germany) and F-actin with phallodin-
Alexa488 (Molecular Probes). Subsequently, slides were washed in PBS,
prior to mounting in Tris/glycerol containing n-propyl-gallate and analyzed
using a Leica DM IRBE fluorescence microscope equipped with a TCSNT
confocal laser system or a Leica DM RXA2 upright microscope, equipped with
a laser scanning confocal head (TCS SP2 AOBS). Conventional
immunofluorescence images were analyzed on a Zeiss Axiovert 100
microscope.
Quantification of α-SMA expression by fluorescence image analysis.
Expression levels of α-SMA in sections of wound granulation tissue were
quantified as described (30). Briefly, sections were triple-immunostained for
α-SMA, desmin and cell nuclei, and confocal digital images were taken using
a Plan-Neofluar 40x/1.3 objective (Zeiss) mounted on a Zeiss Axiovert 200M,
equipped with a spinning disk Nipkow Confocal head (Yokogawa CSU10,
Visitron Systems, Puchheim, Germany), CoolSNAP-HQ monochrome digital
CCD camera (Photometrics, Roper Scientific, Inc., Trenton, NJ) and image
acquisition software (MetaMorph, Universal Imaging Corp. Downington, PA).
Per image a region of interest was manually selected, including the
granulation tissue and all further automatic processing was restricted to this
region. First, desmin-staining, specific for vascular smooth-muscle cells, was
subtracted from α-SMA- and DAPI-images in order to exclude vessels from
α-SMA quantification. Second, α-SMA expression was analyzed by
calculating the mean pixel intensity of the whole region of interest after
background correction and related to the number of cell nuclei obtained from
the desmin-corrected DAPI-image. Tissue was collected from 3 animals per
experimental condition, 3 sections were prepared per animal and 4 regions of
interest were analyzed per section.
by guest on August 17, 2020
http://ww
w.jbc.org/
Dow
nloaded from
9 Thorey et al.
Immunohistochemistry and quantification of blood vessels. For
immunohistochemisty, sections were deparaffinized and treated for 40 min at
room temperature with 1.5% H2O2 in methanol to block endogenous
peroxidases. After a 30 min incubation with 10% rabbit serum, sections were
incubated overnight at 4oC with the PECAM-1 antibody, followed by a 1h
incubation with biotinylated donkey anti-rat IgG (Dianova, Hamburg,
Germany). Detection was performed with the peroxidase substrate kit (Vector
Laboratories, Burlingame, USA), as described by the manufacturer. Sections
were counterstained with hematoxylin, mounted and analyzed using a Zeiss
Axioskop 2 equipped with a Zeiss AxioCam HRc camera. Stained vessels
within an area of 0.2 mm x 0.5 mm below the hyperproliferative epithelium
were counted.
Relaxed and stressed collagen lattice contraction. To determine the effect
of GH on the contractile activity of immortalized embryonic murine fibroblasts
cells were grown in stressed collagen lattice (31) at 1.75x105 cells/ml for 5d
(with our without 1 ng/ml TGF-β1). Attached lattices were then released and
diameter reduction after 30 min was normalized to the initial gel diameter. In
one experimental series, mouse sera and GH were added from the beginning
of the 5d (long-term) culture and in a second series only 5h prior to gel
release (short-term). Tractional cell forces were assessed using relaxed, free-
floating collagen lattices as described (32). 9 x 104 cells/ml gel were seeded
into 6-cm Petri dishes, and collagen gel areas were measured 12 h later. A
minimum of 3 lattices was assayed and experiments were performed in
duplicates.
Acetic acid extraction of proteins from skin. Skin samples were
homogenized in liquid nitrogen and extracted in 1 M acetic acid for 2 h at 4°C.
by guest on August 17, 2020
http://ww
w.jbc.org/
Dow
nloaded from
10 Thorey et al.
Samples were then centrifuged for 5 min at 11.000 g at 4°C and the
supernatant was frozen. Pellets were re-extracted in 1 M acetic acid as
described above. Supernatants were combined and stored at -20°C
overnight. Before determination of protein concentration the samples were
again centrifuged and the supernatants were transferred to fresh tubes, while
the newly formed precipitate was discarded.
Westernblot analysis. 15 µg total protein from lysates of 5-day wounds of
wild-type and transgenic mice were separated by SDS polyacrylamide gel
electrophoresis and transferred to nitrocellulose membranes. Membranes
were probed with primary antibodies against α-SMA and ED-A fibronectin,
stripped and re-probed for total actin using antibody rbAb (Sigma). Detection
was performed with secondary antibodies conjugated to horseradish
peroxidase (Jackson) and the ECL chemiluminescence detection system
(Amersham, Rahn AG, Zürich, Switzerland). Bands were digitized with a
scanner and the ratio between all band densities of one blot was calculated
by commercial computer software (ImageQuant V3.3, Molecular Dynamics,
Sunnyvale, CA). Relative protein expression was normalized to the respective
values for total actin. Samples from 4 animals per experimental condition
were used to calculate mean protein/total actin ratio.
Western ligand blotting. Ligand blot analysis of IGFBPs present in the skin
was performed according to (33), with modifications (34). Briefly, protein
samples were diluted 1:2 with sample buffer (62.5 mM Tris-HCl (pH 6.8), 2%
(w/v) sodium dodecyl sulfate (SDS), 10% (w/v) sucrose), boiled (5 min) and
electrophoresed on a 5% stacking/12% separating SDS-polyacrylamide gel.
Separated proteins were transferred to PVDF membrane (Millipore,
Eschborn, Germany). Blots were blocked with 1% fish gelatin and incubated
with [125I]IGF-II (106 c.p.m. per blot). Binding proteins were visualized and
by guest on August 17, 2020
http://ww
w.jbc.org/
Dow
nloaded from
11 Thorey et al.
quantified using the Phosphor-Imager and the ImageQuant software
(Amersham Biosciences, Freiburg, Germany).
Radioimmunoassays for IGF-I, IGF-II and IGFBP-2. IGF-I, IGF-II and
IGFBP-2 were measured using radioimmunoassays described before (35,
36). For all assays, dilution curves of mouse samples were linear and
paralleled those of human standards.
by guest on August 17, 2020
http://ww
w.jbc.org/
Dow
nloaded from
12 Thorey et al.
Results
bGH transgenic mice show excessive granulation tissue formation and
reduced wound closure at day 5 after wounding. We generated full-
thickness excisional wounds in bGH transgenic mice and control littermates,
and sampled the excised wounds for histological analysis at day 5 after injury
(14 wounds from 7 transgenic males, 12 wounds from 6 wild-type males, 13
wounds from 7 transgenic females and 14 wounds from 7 wild-type females).
At this time point, the inflammatory response is still strong on the one hand,
and on the other hand reepithelialization is already well under way.
Furthermore, part of the clot has been replaced by granulation tissue, which
consists of inflammatory cells, endothelial cells and fibroblasts, which deposit
large amounts of new extracellular matrix (1,2). Fig.1 shows representative
Masson Trichrome stained sections of wounds from transgenic males and
females in comparison to their wild-type littermates. Wounds were much
wider in the transgenic animals of both sexes and filled with a large and cell-
rich granulation tissue (Fig.1A,C,E,G; arrowheads). A large fraction of the
wound was not yet covered by epidermis (Fig.1A,C,E,G; arrows). In the wild-
type animals, on the other hand, the granulation tissue was much less
extended and, therefore, a significant part of the wound was already covered
by newly formed epidermis (Fig.1B,D,F,H; arrows). Finally, the outer margins
of the hyperproliferative epithelium (HE) had moved towards each other due
to contraction of the wounds (Fig.1B,D,F,H; arrowheads).
In addition to the size, the quality of the granulation tissue was also very
different between transgenic mice and control animals: Cells had invaded into
most parts of the original clot and a significant amount of matrix had been
deposited in bGH overexpressing mice (see blue collagen staining). By
contrast, the loose, spongy tissue characteristic for the blood clot was only
partially replaced by granulation tissue in control mice (Fig.1B,D,F). In a few
by guest on August 17, 2020
http://ww
w.jbc.org/
Dow
nloaded from
13 Thorey et al.
wild-type mice, where most of the clot was replaced by granulation tissue at
day 5 after injury (Fig.1H), the granulation tissue was much less extended
compared to transgenic mice.
The oval structures that are detectable in the granulation tissue of some
transgenic animals were identified as hypertrophic nerve fibres after staining
of the sections with an antibody against neurofilament M (data not shown).
They were also detected in most control wounds and to a lesser extent in
wild-type mice of other mouse strains (data not shown). Therefore, they
appear not to be a result of bGH overexpression.
To quantify the histological data, one set of sections from one wounding
experiment (including 5 wounds from 3 transgenic males, 4 wounds from 2
wild-type males, 4 wounds from 2 transgenic females and 5 wounds from 3
wild-type females) was used to measure the cross-sectional area of the
granulation tissue (Fig.2A, encircled area) and the progress of wound closure
(% of distance covered by epidermis between the wound edges which are
indicated by arrowheads in Fig. 1A-H and Fig.2A). Differences in wound
closure (p = 0.0159) and granulation tissue area (p = 0.0317) were significant
in both sexes (Fig.2B,C).
To determine the rate of cell proliferation within the hyperproliferative
epithelium, the animals were injected with bromodeoxyuridine (BrdU) 2 h prior
to sacrifice, and sections from the center of the wounds were stained with an
antibody directed against BrdU. The percentage of stained, proliferating cells
was similar in wild-type and transgenic animals (data not shown). Consistent
with this finding, the area of the HE, as well as its length along the border
between epidermis and dermis, which reflects the rate of keratinocyte
migration, were not significantly different between bGH transgenic and wild-
type mice (data not shown). These results demonstrate that the reduced
wound closure is not the result of delayed reepithelialization, but rather of
by guest on August 17, 2020
http://ww
w.jbc.org/
Dow
nloaded from
14 Thorey et al.
enhanced granulation tissue formation and reduced wound contraction.
Excessive formation of granulation tissue does not lead to a higher
wound bursting strength in bGH transgenic mice. To determine whether
the formation of a larger and denser granulation tissue in the bGH transgenic
animals leads to a functional improvement, we generated incisional wounds
on the back of bGH transgenic and wild-type males and females. Since
incisional wounds are fully healed at day 5 after injury, we sacrificed the
animals at this time point and measured the negative pressure at which the
wounds ruptured. No significant improvement of bursting strength in
transgenic versus wild-type animals was found; rather, the median bursting
strength was slightly higher in both wild-type males and females, compared to
bGH transgenic males and females, respectively (Fig.2D). Similar to the
results from excisional wounds, histology of incisional wounds showed an,
albeit smaller, increase in the density and volume of the granulation tissue
(data not shown). Thus, the excessively dense and thick granulation tissue in
bGH transgenic animals does not function to confer a higher bursting
strength.
Altered neovascularization in 5-day wounds of bGH transgenic animals.
Analysis of Masson trichrome stained sections suggested that the number of
blood vessels is enhanced in bGH transgenic animals. To verify this
impression, we performed immunofluorescence staining on paraffin sections
of 5-day wounds using an antibody against CD31/PECAM (green) combined
with confocal laser scanning microscopy (Fig.3). This staining revealed an
increase in the number and size of newly formed blood vessels (Fig.3A,C),
compared to wounds of wild-type mice (Fig.3B,D). Similar alterations were
observed in transgenic versus wild-type males. To quantify the difference, we
counted the number of blood vessels below the hyperproliferative wound
by guest on August 17, 2020
http://ww
w.jbc.org/
Dow
nloaded from
15 Thorey et al.
epidermis in immunohistochemically stained sections. The difference was
statistically significant (p = 0.0373) in female, but not in male transgenic mice
(p = 0.0703) (Fig.3E). By contrast, we observed a decreased number of blood
vessels within the uninjured skin of transgenic males (data not shown),
demonstrating that bGH alone does not enhance dermal vascularization but
rather requires the presence of additional factors at the wound site to
enhance this process.
In contrast to angiogenesis, no obvious difference in the number of
macrophages was detected between transgenic and wild-type mice as
determined by staining of wound sections with an antibody against the F4/80
antigen (data not shown).
Staining of the keratinocyte-specific markers cytokeratin 14 (Fig.3A-D, red),
cytokeratin 10 (Fig.3A, B; blue-purple) and cytokeratin 6 (data not shown) did
not reveal obvious alterations in keratinocyte differentiation in transgenic as
compared to wild-type animals.
bGH transgenic males show a marked delay in healing at day 13 after
wounding. Fig.4 shows representative Masson Trichrome-stained sections
from 13-day wounds (10 wounds from 6 transgenic males, and 9 wounds
each from 5 wild-type males, 5 transgenic females and 5 wild-type females
were analyzed). At this time point, reepithelialization was completed in wild-
type animals, leaving behind a hyperproliferative epithelium and a granulation
tissue, which both had been greatly reduced in size during the second week
after injury. By contrast, bGH transgenic males (Fig.4A,C) still had an
extensive hyperthickened epithelium, and most notably, 2 of the 10 wounds
analyzed were not yet completely reepithelialized. In wild-type males, on the
other hand, contraction of the wounds had brought the margins of the HE
closely towards each other (arrowheads in Fig.4B,D). Furthermore, in
transgenic males a granulation tissue several times the size of that in wild-
by guest on August 17, 2020
http://ww
w.jbc.org/
Dow
nloaded from
16 Thorey et al.
type animals in height and width was revealed. All transgenic females had
reepithelialized their wounds after 13 days. Very few wounds taken from
transgenic females still had an enlarged wound epithelium and granulation
tissue (Fig.4E); in the majority of these wounds (Fig.4G), the sizes of these
compartments were similar to those found in wild-type females (Fig.4F,H).
The cross-sectional areas of HE and granulation tissue measured in 13-day
wounds are summarized in Fig.4J and K, respectively. For each gender, three
independent wounding experiments were performed, from which data were
compiled and sections through the middle of the wounds were selected (9
wounds from 5 transgenic males, 8 wounds from 5 wild-type males, 5 wounds
from 3 transgenic females and 7 wounds from 5 wild-type females). The
areas were significantly different (HE; p = 0.0003, granulation tissue; p =
0.0025) between transgenic and wild-type males, but not between transgenic
and wild-type females. In accordance with these observations, the percentage
of BrdU-positive proliferating cells, as well as total cell number within the
wound epidermis were still significantly higher in the transgenic males in
comparison to wild-type males (% BrdU positive cells; p = 0.0091, total
number of cells; p = 0.0001), while these parameters were not significantly
different between transgenic and wild-type females. The increased area and
length of the wound epidermis in male animals is most likely due to the
extended granulation tissue that had to be covered, leading to prolonged
keratinocyte hyperproliferation. Consistent with this finding, we found a
prolonged expression of the differentiation-specific keratin 6 in transgenic
males (data not shown).
Taken together, these data indicate that wound closure is delayed in male
and female bGH transgenic mice within the first five days after injury and
even longer in the male animals.
by guest on August 17, 2020
http://ww
w.jbc.org/
Dow
nloaded from
17 Thorey et al.
Altered myofibroblast differentiation and organization of α-smooth
muscle actin (α-SMA) in 5-day wounds of bGH transgenic animals. Of
particular importance for wound contraction and closure is a subpopulation of
fibroblasts that differentiate into myofibroblasts during the course of wound
healing (37). To investigate whether the obvious defect in wound contraction
in the bGH transgenic animals is due to alterations in myofibroblast
differentiation, sections were stained for α-SMA, which is expressed by
myofibroblasts. In wounds from wild-type females, a highly organized
structure of α-SMA-containing stress fibers underlying the hyperproliferative
epithelium was revealed (Fig.5B,D; green), with filaments extending along the
hyperproliferative wound epithelium and also underneath the uninjured
dermal tissue at the edge of the wound towards the subcutaneous muscle,
the panniculus carnosus. The latter can be identified on the basis of strong
desmin staining (red). In the granulation tissue, α-SMA expressing cells could
unmistakably be identified as myofibroblasts (green), since they were
negative for desmin in contrast to smooth muscle cells of small vessels, which
co-express α-SMA and desmin (Fig.5C,D, yellow, indicated by arrows).
However, in wounds from transgenic females, fewer myofibroblasts residing
underneath the keratinocyte tongues at the wound edges expressed much
less α-SMA, most of which was not organized into parallel filaments but rather
extended in all directions (Fig.5A,C; green). A similar difference was also
seen in male mice (data not shown). Quantification of myofibroblast
appearance in granulation tissue by immunofluorescence intensity analysis of
5d wound sections demonstrated approximately 3-times higher α-SMA
expression in female wild-type compared to transgenic mice. This was
confirmed by Westernblot analysis of total lysates of 5-day wound tissue
(Fig.6A,B), revealing a 3-fold and 2.5-fold higher expression of α-SMA in wild-
type male and female mice compared to their respective transgenic
littermates. A second marker for myofibroblasts, ED-A fibronectin (38) was
by guest on August 17, 2020
http://ww
w.jbc.org/
Dow
nloaded from
18 Thorey et al.
expressed at significantly higher levels in wild-type (4-fold) compared to
transgenic female mice, but exhibited similar expression levels in male
transgenic and control mice. These results suggest that impaired wound
contraction in bGH transgenic animals correlates with a decreased number of
myofibroblasts and an impairment of stress fiber organization in wound
myofibroblasts.
Effect of bGH on collagen contraction and myofibroblast differentiation.
As a next step we determined whether the impaired wound contraction, which
we observed in bGH-overexpressing transgenic mice, is a direct effect of GH
on the generation of contractile and tractional forces by fibroblasts. For this
purpose we analyzed the effect of recombinant bGH on the ability of murine
embryonic fibroblasts to contract attached (stressed) three-dimensional
collagen lattices, which are a model of the organized matrix in advanced
granulation tissue (37), and to retract freely floating (relaxed) gels, in which
loose collagen fibrils are reorganized by migrating fibroblasts (39),
comparable to early dermal wound healing. The GH concentrations that we
used ranged from 0.1% - 10% of the serum concentrations of bGH transgenic
mice, and therefore likely reflect the concentrations that reach the fibroblasts
within the dense granulation tissue. When GH was added for 5h to attached
(Fig.7A, control) and 12h to free-floating gels (data not shown) in control
medium, we did not observe any inhibitory effect of GH on collagen area
reduction, but rather a tendency of this hormone to enhance
contraction/retraction in a dose-dependent manner. As a next step, we
determined if growth hormone affects myofibroblast differentiation and the
contractile ability of these cells. For thus purpose, fibroblasts were cultured
for 5 days in the presence of transforming growth factor β1 (TGF-β1). This
factor was chosen, since TGF-βs are the most potent known inducers of
myofibroblast differentiation (31, 40), and since TGF-β1 is the predominant
by guest on August 17, 2020
http://ww
w.jbc.org/
Dow
nloaded from
19 Thorey et al.
TGF-β isoform in murine skin wounds (41). When fibroblasts were grown for
5d in stressed gels in the presence of TGF-β1, i.e. when myofibroblast
differentiation has been induced, short-term addition of GH moderately
decreased myofibroblast contractile activity (Fig.7A, TGF-β1). Interestingly,
addition of GH for the whole culture period of 5d had no effect on stressed
collagen contraction in control medium (Fig.7C, control), but significantly
reduced the contractile activity of (myo)fibroblasts grown in the presence of
TGF-β1 (Fig.7C, TGF-β1).
Next, we tested the possibility that the serum of bGH transgenic mice
contains an inhibitory activity, which counteracts the positive short-term
influence of GH on fibroblast collagen gel reduction. In control medium,
replacement of 5% FCS with pooled sera of transgenic or wild-type mice
resulted in an improvement of gel retraction (data not shown) and contraction
when added for 5h (Fig.7B, control) and 5d (Fig.7D, control); this effect is
presumably due to the greater efficiency of murine over bovine growth
factors. At lower concentrations of mouse sera the degree of collagen gel
retraction was intermediate between the control and the 5% mouse serum
values, but no significant difference was seen between sera from transgenic
or wild-type mice at any concentration tested (data not shown). When added
to TGF-β1-treated (myo)fibroblasts, serum from transgenic mice slightly
reduced stressed collagen contraction compared to 10% FCS and wild-type
mouse serum (Fig.7B, D, TGF-β1).
To assess the level of myofibroblast differentiation, murine embryonic
fibroblasts were treated for 5d with TGF-β1 in the presence or absence of
bGH or mouse sera. TGF-β1 strongly induced expression of α-SMA (Fig.7E),
compared to almost α-SMA-negative cells grown in control medium (data not
shown). This α-SMA-inducing effect of TGF-β1 was completely abolished by
simultaneously adding GH (Fig.7F) and moderately reduced by transgenic
mouse serum (Fig.7H); wild-type mouse serum did not change α-SMA
by guest on August 17, 2020
http://ww
w.jbc.org/
Dow
nloaded from
20 Thorey et al.
expression of TGF-β1-treated fibroblasts (Fig.7G). When added to fibroblasts
in control medium, GH and mouse sera had no significant effect on α-SMA
expression (data not shown).
Thus in long-term experiments, GH appears to inhibit TGF-β1-induced
myofibroblast differentiation and α-SMA expression, which is most likely
responsible for reduced collagen (31) and wound contraction. Moreover, in
short-term treatment, GH seems to inhibit the contractile activity of
differentiated myofibroblasts but not the retraction forces exerted by α-SMA-
negative fibroblasts.
Elevated levels of IGFBPs, but not of IGF-I, in 5-day wounds of bGH
transgenic mice. Since many effects of GH are mediated via IGFs, we
compared the levels of IGF and IGF binding activities in skin and wound
lysates derived from bGH transgenic mice and wild-type mice. IGF-I levels in
protein lysates prepared from individual mice (n=4) were determined by
quantitative radioimmunoassay (Fig.8A). As reported previously for serum
IGF-I levels (27), they were elevated by a factor of 2-3 in transgenic skin of
both males and females, compared to wild-type (males; p = 0.0006, females;
p = 0.0008). In the females, a 6-fold upregulation of IGF-I protein in
comparison to non-wounded skin was observed in both wild-type and
transgenic animals at day 5 after injury; however, no difference was observed
between transgenic and wild-type animals. Much less upregulation of IGF-I
was observed in the males; levels in 5-day-wounds of both wild-type and
transgenic males were similar to those in the uninjured skin of transgenic
males. The difference between males and females was highly significant for
both wild-type (p = 0.0037) and transgenic (p = 0.0025) mice. Thus, first, IGF-
I levels seem to be generally lower in healing wounds of male mice,
compared to females; and second, in bGH transgenic mice of both genders,
the higher abundance of IGF-I in intact skin of transgenic mice compared to
by guest on August 17, 2020
http://ww
w.jbc.org/
Dow
nloaded from
21 Thorey et al.
wild-type mice is not maintained after injury . When levels of IGF-II and
IGFBP-2 within the same samples were determined, no significant differences
were revealed between wild-type and bGH transgenic mice (data not shown).
IGF binding activities in skin and 5-day wounds were analyzed by western
ligand blotting of protein lysates from individual mice (n = 3 for each gender
and genotype) with a radiolabelled IGF-II tracer (Fig.8B). Three labelled
bands visualized on the blots corresponded to IGFBP-3 (35-45 kDa), IGFBP-
5 (25-35 kDa) and IGFBP-4 (18-25 kDa), the three IGF binding proteins,
which are expressed mainly by dermal fibroblasts (18, 42). An increase in IGF
binding to all three proteins could be observed in skin lysates from both
transgenic males and females, compared to wild-type animals; this increase
was significant for IGFBP-3 in both genders (males; p = 0.0085, females; p =
0.0013) and for IGFBP-4 in the females (p = 0.017), and not significant in the
other skin samples, due to larger variations between the individuals.
Following injury, IGF binding activity was upregulated (2-4-fold in the wild-type
animals and 1.5-3-fold in bGH transgenic mice). In 5-day wound lysates, a
significant difference was observed between wild-type and bGH transgenic
mice in binding to both IGFBP-3 (males; p = 0.0052, females; p= 0.025) and
IGFBP-4 (males; p = 0.0014, females; p = 0.0008), while no difference was
apparent in binding to IGFBP-5. Thus, overall in the wounds of bGH
transgenic mice the balance between IGFs and IGFBPs is shifted towards an
under-abundance of IGF-I and a greater relative activity of the predominantly
inhibitory IGF binding proteins, IGFBP-3 and IGFBP-4.
by guest on August 17, 2020
http://ww
w.jbc.org/
Dow
nloaded from
22 Thorey et al.
Discussion
Growth hormone: beneficial or detrimental for wound healing? We have
studied the wound healing process in transgenic mice with highly elevated
levels of serum bGH. The most striking phenotype was the strong increase in
granulation tissue formation in female and male transgenic animals. This
result is consistent with data obtained by other investigators who found that
local or systemic application of GH stimulates granulation tissue formation in
wounds of normal and malnourished rats (8, 43). However, in the latter and in
other studies (9), the increased granulation tissue correlated with an improved
biomechanical strength of the wounds. By contrast, we could not detect an
increase in wound bursting strength, demonstrating that matrix maturation is
not improved by the elevated levels of bGH. These discrepancies between
our results and previous studies might result from the use of healing-impaired
animals in most treatment studies. These animals suffer from reduced
mechanical wound strength, which is likely to be improved by application of
GH. However, we show that GH is not able to further increase the normal
bursting strength of a non-compromised wound and can even delay the
wound healing process. Thus, GH treatment of healthy individuals appears to
have adverse effects on skin wound healing. On the other hand, GH was
found to be helpful in severely burned animals or patients, who are
characterized by the induction of a catabolic state with decreased GH and
IGF levels. In this case the action of exogenously administered GH may lie
more in the restoration of the anabolic metabolism, rather than in the
stimulation of tissue repair at the cellular level (7).
Enhanced wound angiogenesis in bGH transgenic mice. A remarkable
feature of the granulation tissue of bGH transgenic mice was the increased
number of blood vessels. This may be a direct effect of GH, since the latter
was shown to stimulate angiogenesis (44, 45). However, GH alone is not
by guest on August 17, 2020
http://ww
w.jbc.org/
Dow
nloaded from
23 Thorey et al.
sufficient to stimulate this process in the skin, since the number of blood
vessels in unwounded skin of bGH transgenic males was even reduced.
Thus, additional factors present at the wound site are likely to contribute to
the increased angiogenesis. Possible candidates are VEGF, IGF-I and TGF-
β1, angiogenic factors which are overexpressed in skin wounds (2). These
growth factors might act synergistically with GH to stimulate angiogenesis. By
contrast, they are probably not directly responsible for the increase in vessel
number and size, since their expression was not enhanced in wounds of bGH
transgenic mice compared to control animals (data not shown). Furthermore,
IGF-I activity in wounded skin of bGH mice appears even reduced due to the
enhanced expression of inhibitory IGFBPs at the wound site. Therefore, the
stimulatory effect of GH on granulation tissue formation is most likely not
mediated via IGF-I.
Abnormal wound contraction and myofibroblast differentiation in bGH
transgenic mice. The most striking abnormality in the bGH transgenic mice
was the inefficient wound contraction, leading to a delay in wound closure,
which is more pronounced in the males than in the females. It has been
suggested that the initial closure of the wound is due to tractional forces that
are developed by migrating fibroblasts (46). This process can be mimicked in
vitro using free-floating collagen lattices, where the reduction in collagen
lattice diameter is entirely due to tractional forces exerted by fibroblasts (39).
However, collagen gel retraction in vitro was even enhanced by recombinant
bGH and by serum from bGH transgenic mice. The positive effect may result
from the induction of IGF-I expression in fibroblasts by bGH, since IGF-I is
known to promote fibroblast-mediated collagen gel contraction (47, 48).
At later stages of wound healing, a subpopulation of fibroblasts differentiates
into myofibroblasts, which are thought to be responsible for contraction of the
granulation tissue (37). Remarkably, a strongly reduced number of
by guest on August 17, 2020
http://ww
w.jbc.org/
Dow
nloaded from
24 Thorey et al.
myofibroblasts was observed in bGH transgenic mice, and the existing
myofibroblasts showed a decrease in the abundance of parallel α-SMA
containing stress fibers. This finding suggests that the contractile capability of
the existing myofibroblasts is impaired. Of particular importance for
myofibroblast differentiation is TGF-β1 (40). The normal expression of this
growth and differentiation factor in bGH transgenic mice suggests that
alterations in the levels of TGF-β1 are not responsible for the defect in
myofibroblast differentiation. By contrast, our in vitro studies with stressed
three-dimensional collagen lattices revealed that GH reduces the contractile
activity of (myo)fibroblasts grown in the presence of TGF-β1. Consistent with
this observation, TGF-β1-induced myofibroblast differentiation in vitro was
strongly inhibited by long-term treatment with bGH. This result revealed a
novel role of GH as an inhibitor of TGF-β-induced myofibroblast differentiation
and suggests that this hormone also impairs TGF-β-induced myofibroblast
differentiation and the contractile capacity of these cells in wounded skin.
Interaction of growth hormone with androgens at the wound site?
Interestingly, the enlarged, highly vascularized granulation tissue and the
myofibroblast abnormalities were observed in both male and female
transgenic mice. This finding demonstrates that the abnormalities seen in
early wounds are not a result of the highly fibrotic skin of male transgenic
animals, which could impair wound contraction. Rather, bGH appears to
affect granulation tissue formation in mice of both genders in a similar
manner. However, the phenotype was stronger in the male animals, possible
due to the influence of sexual hormones as already observed in non-injured
skin of these animals (26). In this study, the severe skin fibrosis seen in male
animals was prevented when the animals were castrated, demonstrating that
androgens synergize with GH and possibly locally acting growth factors to
induce skin fibrosis. In analogy, the continuous production of matrix at the
by guest on August 17, 2020
http://ww
w.jbc.org/
Dow
nloaded from
25 Thorey et al.
wound site and the extension of the inflammatory phase (data not shown)
could also be influenced by androgens. This hypothesis is supported by
findings from Ashcroft and Mills (5), who found that testosterone is a negative
regulator of wound healing and enhances the inflammatory response by up-
regulation of pro-inflammatory cytokines.
In summary, we have shown striking effects of enhanced serum GH levels on
the wound healing process. In addition to its known effect on granulation
tissue formation, our results revealed a novel role of GH in wound
angiogenesis. Most interestingly, GH was identified as an inhibitor of TGF-β-
induced myofibroblast differentiation. Finally, our data strongly suggest that
systemic GH treatment is detrimental for wound healing in non-healing
impaired individuals, in particular in males.
by guest on August 17, 2020
http://ww
w.jbc.org/
Dow
nloaded from
26 Thorey et al.
Acknowledgements
We thank C. Born-Berclaz and J. Smith-Clerc for excellent technical
assistance and Dr. Luciano Zardi (National Institute for Cancer Research,
Laboratory of Cell Biology, Genova, Italiy) for providing the IST-9 antibody.
Dr. J.-J. Meister is gratefully acknowledged for his constant support of the
work of B.H. and for providing lab facilities at the EPFL. This work was
supported by grants from the Swiss National Science Foundation (No. 31-
61358.00 to S.W. and No.3100A0-102150/1 to B.H) and the German Ministry
for Education and Research (BMBF) (to S.W. and E.W.).
by guest on August 17, 2020
http://ww
w.jbc.org/
Dow
nloaded from
27 Thorey et al.
References
1. Martin, P. (1997) Science 276, 75-81
2. Werner, S., and Grose, R. (2003) Phys. Rev. 83, 835-870
3. Ashcroft, G.S., Dodsworth, J., van Boxtel, E., Tarnuzzer, R.W., Horan,
M.A., Schultz, G.S., and Ferguson, M.W. (1997) Nat. Med. 3, 1209-
1215
4. Grose, R., Werner, S., Kessler, D., Tuckermann, J., Huggel, K., Durka,
S., Reichardt, H.M., and Werner, S. (2002) EMBO reports 3: 575-582.
5. Ashcroft, G.S., and Mills, S.J. 2002. J. Clin. Invest. 110, 615-624
6. Cummings, D.E., and Merriam. G.R. (2003) Annu Rev Med. 54, 513-
533.
7. Lal, S.O., Wolf, S.E., and Herndon, D.N. (2000) Growth Horm. IGF
Res. 10, Suppl. B, S39-S43
8. Steenfos, H.H. and Jansson, J.O. (1992) J. Endocrinol. 132, 293-298
9. Seyer-Hansen, M., Andreassen, T.T., Jorgensen, P.H., and Oxlund, H.
(1993) Eur. Surg. Res. 25, 162-168
10. Rasmussen, L.H., Garbarsch, C., Schuppan, D., Moe, D., Horslev-
Pedersen, K., Gottrup, F., and Steenfos, H. (1995) Eur. J. Surg. 161,
157-162
11. Ghofrani, A., Holler, D., Schuhmann, D., Saldern, S., and Messmer,
B.J. (1999) Plast. Reconstr. Surg. 104, 470-475.
12. Seyer-Hansen, M., Andreasen, T.T., and Oxlund, H. (1999) Growth
Horm. IGF Res. 9, 254-261
13. Welsh, K.M., Lamit, M., and Morhenn, V.B. (1991) J. Invest. Surg.
Oncol. 17, 942-945
14. Green, H., Morikawa, M., and Nixon, T. (1985) Differentiation 29, 195-
198
15. Eming, S.A, Snow, R.G., Yarmush, M.L., and Morgan, J.R. (1996) J.
by guest on August 17, 2020
http://ww
w.jbc.org/
Dow
nloaded from
28 Thorey et al.
Invest. Dermatol. 107, 113-120
16. Martin, J.L., and Baxter, R.C. (1999) in Contemporary Endocrinology;
The IGF System. (Rosenfeld, R., and Roberts, C., eds) pp. 227-254,
Humana Press, Inc. Totowa, NJ
17. Kuroda, K., Utani, A., Hamasaki, Y. and Shinkai, H. (2001) J.
Dermatol. Sci. 26, 156-160
18. Clemmons, D.R. (1999) in Contemporary Endocrinology; The IGF
System. (Rosenfeld, R., and Roberts C. jr., eds) pp. 273-279, Humana
Press, Inc. Totowa, NJ
19. Schneider, M.R., Wolf, E., Hoeflich, A., and Lahm. H. (2002) J.
Endocrinol. 172, 423-440
20. Lynch S,E., Colvin, R.B. and Antoniades, H.N. (1989) J. Clin. Invest.
84, 640-646
21. Jyung, R.W., Mustoe, J.A., Busby, W.H., and Clemmons, D.R. (1994)
Surgery 115, 233-239.
22. Bitar, M.S. (1997) Horm. Metab. Res. 29, 383-386
23. Jeschke, M.G., Barrow, R.E., Hawkins, H.K., Yang, K., Hayes, R.L.,
Lichtenbelt, B.J., Perez-Polo, J.R., and Herndon, D.N. (1999) Gene
Ther. 6, 1015-1020
24. Dunaiski, V., and Belford, D.A. (2002) Growth Hormone IGF Res. 12,
381-387
25. Wolf, E., and Wanke, R. (1996) in Welfare of Transgenic Animals.
Zutphen, L.F.M., and van der Meer, M., eds) pp. 26-47, Springer
Verlag. Heidelberg, Germany
26. Wanke, R., Milz, S., Rieger, N., Ogiolda, L., Renner-Muller, I., Brem,
G., Hermanns, W., and Wolf, E. (1999) J. Invest. Dermatol. 113, 967-
971.
27. Hoeflich, A., Nedbal, S., Blum, W.F., Erhard, M., Lahm, H., Brem, G.,
Kolb, H.J., Wanke, R., and Wolf, E. (2001) Endocrinol. 142, 1889-1898
by guest on August 17, 2020
http://ww
w.jbc.org/
Dow
nloaded from
29 Thorey et al.
28. Skalli, O., Ropraz, P., Trzeciak, A., Benzonana, G., Gillessen, D., and
Gabbiani, G. (1986). J. Cell Biol. 103, 2787-2796.
29. Borsi, L., Carnemolla, B., Castellani, P., Rosellini, C., Vecchio, D.,
Allemanni, G., Chang, S.E., Taylor-Papadimitriou, J., Pande, H., and
Zardi, L. (1987). J. Cell Biol. 104, 595-600.
30. Hinz, B., Mastrangelo, D., Iselin, C.E., Chaponnier, C., and Gabbiani,
G. (2001) Am. J. Pathol. 159, 1009-1020.
31. Hinz, B., Celetta, G., Tomasek, J.J., Gabbiani, G., and Chaponnier, C
(2001a). Mol. Biol. Cell 12, 2730-2741
32. Kessler, D., Dethlefsen, S., Haase, I., Plomann, M., Hirche, F., Krieg,
T., and Eckes, B. (2001) J. Biol. Chem. 276, 36575-36585
33. Hossenlopp, P., Seurin, D., Segovia Quinson, B., Hardouin, S., and
Binoux, M. (1986) Anal. Biochem. 154, 138-143.
34. Wolf, E., Kramer, R., Blum, W. F., Foll, J., and Brem, G. (1994)
Endocrinol. 135, 1877-1886
35. Bang, P., Baxter, R. C., Blum, W. F., Breier, B. H., Clemmons, D. R.,
Hall, K., Hintz, R. L., Holly, J. M., Rosenfeld, R. G., and Zapf, J. (1994)
J.Endocrinol. 143, C1-2
36. Hoeflich, A., Wu, M., Mohan, S., Föll, J., Wanke, R., Froehlich, T.,
Arnold, G., Lahm, H., Kolb, H. J., and Wolf, E. (1999) Endocrinol. 140,
5488-5496
37. Tomasek, J.J., Gabbiani, G., Hinz, B., Chaponnier, C. and Brown, R.A.
(2002) Nat. Rev. Mol. Cell Biol. 3, 349-363
38. Serini, G., Bochaton-Piallat, M.L., Ropraz, P., Geinoz, A., Borsi, L.,
Zardi, L., and Gabbiani, G. (1998). J. Cell Biol. 142, 873-881
39. Bell, E., Ivarsson, B., and Merrill, C. (1979) Proc. Natl. Acad. Sci. USA
76, 1274-1278
40. Desmouliere, A., Geinoz, A., Gabbiani, F., and Gabbiani, G. (1993) J.
Cell. Biol. 122, 103-111
by guest on August 17, 2020
http://ww
w.jbc.org/
Dow
nloaded from
30 Thorey et al.
41. Frank, S., Madlener, M., and Werner, S. (1996). J. Biol. Chem. 271,
10188-10193
42. Giannini, S., Mohan, S., Kasuya, J., Galli, G., Rotella, C.M., LeBon,
T.R., and Fujita-Yamaguichi, Y. (1994) J. Clin. Endocrinol. Metabol. 79,
1824-1830
43. Zaizen, Z., Ford, E.G., Shimada, H., Kosi, M., Costin, G., and Atkinson,
J.B. (1995) Eur. J. Pediatr. Surg. 5, 226-230
44. Gould, J., Aramburo, C., Capdevielle, M., and Scanes, C.G. (1995) Life
Sci. 56, 587-594
45. Struman, I., Bentzien, F., Lee, H., Mainfroid, V., D'Angelo, G., Goffin,
V., Weiner, R.I., and Martial, J.A. (1999) Proc. Natl. Acad. Sci. USA
96, 1246-12451
46. Ehrlich, H.P., and Rajaratnam, J.B. (1990) Tissue Cell 22, 407-417
47. Lee, Y.R., Oshita, Y. and Tsuboi, R. (1996) Endocrinol. 137, 5378-
5283
48. Kanekar, S., Borg, T.K., Terracio, and L., Carver, W. (2000) Cell
Adhes. Commun. 7, 513-523.
by guest on August 17, 2020
http://ww
w.jbc.org/
Dow
nloaded from
31 Thorey et al.
Figure legends
Fig. 1. Impaired wound healing in bGH overexpressing transgenic mice.
Masson Trichrome stained paraffin sections from the center of 5-day wounds
of bGH overexpressing transgenic males (A,C) and females (E,G) and their
male and female wild-type littermates (B,D; and F,H; respectively). Shown are
low-magnification views of representative wounds. Arrows indicate the
foremost tips of the epithelial tongues. Arrowheads indicate the wound edges.
D, dermis; E, epidermis; Es, eschar; G, granulation tissue; HE,
hyperproliferative epithelium; M, muscle (Panniculus carnosus). Note the
extensive skin fibrosis in transgenic males, and the increased granulation
tissue in all transgenic animals. Bars represent 1 mm.
Fig. 2. Delayed wound closure, enlarged granulation tissue, but no
improvement of wound bursting strength in wounds of bGH transgenic
mice. A set of representative sections from full-thickness excisional wounds
(Fig.1) was subjected to morphometric analysis as illustrated in A. The area of
granulation tissue, which was measured, is encircled by a black line. Wound
closure was determined as percentage of distance covered by epidermis
between the wound edges which are indicated by arrowheads in Fig. 1A-H,
Fig. 2A). B,C: Both the percentage of wound closure (J; p=0.159) and the
area of granulation tissue/fibrin clot (K; p=0.317) were significantly different
between transgenic and wild-type males as well as between transgenic and
wild-type females (open circles). Shown are single data points for each
wound and median. *p<0.05. D: Incisional wounds were created on the back
of bGH transgenic and wild-type mice 5 days prior to post-mortem
measurement of bursting strength using a suction device. Shown are median
values, 25th to 75th percentile (box) and range (vertical bars) of males (19
transgenic; 50 wild type) and females (20 transgenic; 26 wild type).
by guest on August 17, 2020
http://ww
w.jbc.org/
Dow
nloaded from
32 Thorey et al.
Differences between the four groups are not significant. Note the extended
upper range of wild-type wound bursting strength, presumably reflecting
completed reepithelialization of some wounds.
Fig. 3. Enhanced angiogenesis in bGH transgenic mice. A-D: Paraffin
sections prepared from 5-day wounds of bGH transgenic mice or their wild-
type siblings were triple-stained with a polyclonal antiserum against
cytokeratin 14, followed by Cy-3 conjugated anti-rabbit IgG (red); a rat
monoclonal antibody against CD 31/PECAM, followed by FITC-conjugated
anti-rat-IgG (green), and a mouse monoclonal antibody against cytokeratin
10, followed by Cy-5 conjugated anti-mouse IgG (blue; signal throughout the
fibrin clot/granulation tissue probably represents binding to mouse serum
IgGs). Shown are low-magnification views of representative wound edges
(A,B, bars represent 100 µm) and higher magnification views of areas of the
fibrin clot/granulation tissue underlying the hyperproliferative epithelium (C,D,
bars represent 20 µm). D, dermis; E, epidermis; G, granulation tissue; HE,
hyperproliferative epithelium. E: Quantification of blood vessels below the
hyperproliferative epithelium in sections from female transgenic mice (10
wound halves) and control animals (5 wound halves) and from male
transgenic mice (8 wound halves) and control animals (5 wound halves)
revealed a significantly higher number of vessels in transgenic females
compared to controls (p= 0.0373), whereas the difference was not significant
in males (p = 0.0703). Shown are median values, 25th to 75th percentile (box)
and range (vertical bars).
Fig. 4. Severely delayed wound healing in bGH overexpressing males.
Masson-Trichrome stained paraffin sections from the center of 13-day
wounds from bGH transgenic males (A,C) and females (E, G) and their male
and female wild-type siblings (B,D; and F,H; respectively). Shown are low-
by guest on August 17, 2020
http://ww
w.jbc.org/
Dow
nloaded from
33 Thorey et al.
magnification views of typical wounds. Panel A shows a wound with
incomplete closure; arrows indicate the foremost tips of the epithelial tongues.
Arrowheads in all panels indicate the wound edges. D, dermis; E, epidermis;
G, granulation tissue; HE, hyperproliferative epithelium; M, muscle
(Panniculus carnosus). Note the enlarged granulation tissue of the transgenic
males and of one transgenic female. Bars represent 1 mm.
J,K: A set of representative sections was subjected to morphometric analysis
which revealed highly significant differences in the areas of the
hyperproliferative epithelium (J; p=0.0003) and the granulation tissue (K;
p=0.0025) between transgenic males (filled squares) and wild-type males
(open squares), while differences between transgenic females (filled circles)
and wild-type females (open circles) were not significant. Shown are single
data points for each wound, and median. **p<0.01; ***p<0.001
Fig.5. Altered myofibroblast differentiation in bGH transgenic mice.
Paraffin sections prepared from 5-day wounds of bGH transgenic mice or
their wild-type siblings were triple-stained with a polyclonal antiserum
against cytokeratin 14 followed by Alexa647-conjugated anti-rabbit IgG (A-
D, blue), a mouse monoclonal IgG2a antibody against α-SMA (green)
followed by FITC-conjugated anti-mouse IgG2a and a mouse monoclonal
IgG1 antibody against desmin (red) followed by TRITC-conjugated anti-
mouse IgG1. Sections were viewed by laser confocal microscopy and
overlays were prepared from the extended-view images from all three
channels. Shown are low-magnification views of representative wound
edges (A,B,: bars represent 100 µm) and higher magnification views of
areas of the fibrin clot/granulation tissue underlying the hyperproliferative
epithelium (C,D; bars represent 20 µm). D, dermis; E, epidermis; G,
by guest on August 17, 2020
http://ww
w.jbc.org/
Dow
nloaded from
34 Thorey et al.
granulation tissue; HE, hyperproliferative epithelium. M in panels A, B
indicates the position of the subcutaneous muscle (panniculus carnosus)
and arrowheads (C, D) point to small vessels.
Fig.6. Expression of myofibroblast marker proteins is down-regulated
in bGH transgenic mice. (A) Expression of total actin and the
myofibroblast markers ED-A fibronectin and α-SMA was determined by
Western blotting on total lysates, prepared from 5-day wounds of bGH
transgenic (tg) male and female mice and their wild-type littermates (wt).
Protein loads have been equilibrated for vimentin expression levels. (B)
Protein bands were scanned, quantified by image analysis and normalized
to total actin. Results are presented as mean values ± standard deviation.
Significance was tested by means of a two-taled heteroscedastic
Student`s t-test. Differences were considered to be statistically significant
at values of p<0.05. In contrast to largely unchanged levels of total actin,
expression of α-SMA is significantly reduced in transgenic compared to
wild-type mice. ED-A fibronectin (ED-A FN) is significantly reduced in
female but not in male transgenic mice compared to their respective wild-
type littermates (**p<0.01).
Fig. 7. Effects of bGH and transgenic mouse serum on stressed
collagen gel contraction and myofibroblast differentiation.
Immortalized mouse fibroblasts were seeded into mechanically stressed,
attached collagen gels and grown for 5d in normal medium (control) and
medium, containing 1 ng/ml TGF-β1 (TGF-β1) in order to induce
by guest on August 17, 2020
http://ww
w.jbc.org/
Dow
nloaded from
35 Thorey et al.
myofibroblast differentiation. Gels were additionally treated with different
concentrations of bGH (12.3 ng/ml, 61.3 ng/ml, or 245 ng/ml) (A, C) or 5%
FCS + 5% pooled sera from wild-type mice; or from their bGH transgenic
siblings (bGH levels in pooled sera from transgenic mice were 1.6 µg/ml)
(B, D). Treatment was either short-termed (5h, A, B) or performed during
the whole culture period of 5d (C, D). After 5d, attached gels were
released and area reduction after 30 min was normalized to control
contraction (10% FCS). Indicated in column charts: *p ≤ 0.05, **p ≤ 0.01,
***p ≤ 0.001 as tested by means of a two-tailed heteroscedastic Student's
t-test within one experimental condition (control, TGF-β1) against the
respective 0-value (A,C) or between wt and tg contraction (B, D); n=3.
After 5d culture in medium containing 1 ng/ml TGF-β1 (E) and additionally
245 ng/ml bGH (F), 5% serum from wild-type mice + 5% FCS (G) or 5%
serum from transgenic mice + 5% FCS (H), cells were stained for α-SMA
(red), F-actin (phalloidin, green) and nuclei (DAPI, blue) to determine the
level of myofibroblast differentiation. Note that bGH significantly reduces
the level of α-SMA expression. Bar: 50 µm.
Fig. 8. Altered balance between IGF-I and IGFBPs in wounds of bGH
transgenic mice. Levels of IGF-I in total protein lysates prepared from
uninjured skin and 5-day wounds (5d W) of bGH transgenic males and
females and their wild-type littermates were determined by quantitative
radioimmunoassay, and means and SEM were calculated (A). Significant
differences were revealed between transgenic and wild-type skin of both
males (p =0.0006) and females (p = 0.0008).
Aliquots of total protein lysates from uninjured skin and 5-day wounds of bGH
transgenic males and females and their wild-type littermates were subjected
by guest on August 17, 2020
http://ww
w.jbc.org/
Dow
nloaded from
36 Thorey et al.
to Western ligand blot analysis using radiolabelled IGF-II tracer (B,C). Binding
activity was determined separately for 3 different samples per gender,
genotype and condition in one experiment, and means and SEM were
calculated (B). IGFBP-3 binding was significantly different between transgenic
and wild-type animals in the skin of males (p = 0.0085) and females (p =
0.0013), as well as in 5-day wounds of males (p = 0.0052) and females (p =
0.025). IGFBP-4 binding was significantly different between transgenic and
wild-type animals in the skin of the females only (p = 0.017), and in 5-day
wounds of both males (p = 0.0014) and females (p = 0.0008). As an example,
the image of a ligand blot prepared in a different experiment with 5-day
wound samples of females is also shown (C). 3, 4, 5 indicates the positions of
the bands corresponding to IGFBP-3, IGFBP-5, and IGFBP-4. Note that the
medium-size band in the serum positive control (S), which corresponds to
IGFBP-2, does not co-migrate with IGFBP-5. *p<0.05, **p<0.01; ***p<0.001.
by guest on August 17, 2020
http://ww
w.jbc.org/
Dow
nloaded from
Martin Elmlinger, Ruediger Wanke, Eckhard Wolf and Sabine WernerIrmgard S. Thorey, Boris Hinz, Andreas Hoeflich, Susanne Kaesler, Philippe Bugnon,
angiogenesis and myofibroblast differentiationTransgenic mice reveal novel activities of growth hormone in wound repair,
published online April 7, 2004J. Biol. Chem.
10.1074/jbc.M311467200Access the most updated version of this article at doi:
Alerts:
When a correction for this article is posted•
When this article is cited•
to choose from all of JBC's e-mail alertsClick here
by guest on August 17, 2020
http://ww
w.jbc.org/
Dow
nloaded from