effects of rho-kinase inhibition on established … · cor pulmonale and eventual death. the...
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EFFECTS OF RHO-KINASE INHIBITION ON ESTABLISHED
CHRONIC HYPOXIC PULMONARY HYPERTENSION IN THE
NEONATAL RAT
By
Emily Zhi Xu, H.B.Sc.
A thesis submitted in conformity with the requirements for the degree of Master of Science
Graduate Department of Physiology
University of Toronto
© Copyright Emily Zhi Xu (2010)
ii
ABSTRACT
Effects of Rho-kinase inhibition on established chronic hypoxic pulmonary hypertension
in the neonatal rat.
Emily Zhi Xu, M.Sc, 2010
Department of Physiology, School of Graduate Studies
University of Toronto, Canada
Rationale: Vascular remodeling and right-ventricular (RV) dysfunction are features of
refractory pulmonary hypertension (PHT) in human neonates. These features are replicated in
rats chronically exposed to hypoxia (13% O2), in which increased pulmonary vascular resistance
(PVR) was acutely normalized by Y-27632, a Rho-kinase (ROCK) inhibitor, but not by inhaled
nitric oxide.
Objective: To examine the reversing effects of sustained ROCK inhibition on haemodynamic
(RV dysfunction and increased PVR) and structural (RV hypertrophy and arterial wall
remodeling) changes of chronic hypoxic PHT.
Methods: Rat pups were exposed to air or hypoxia from birth for up to 21 days and received Y-
27632 (15 mg/kg/b.i.d.) or vehicle from day 14.
Results: Y-27632 normalised RV dysfunction and reversed remodeling secondary to chronic
hypoxia. These changes were accompanied by increased apoptosis of smooth muscle and
attenuated endothelin-1 expression in pulmonary arteries.
Conclusion: ROCK inhibitors hold promise as a rescue therapy for refractory PHT in neonates.
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ACKNOWLEDGEMENTS
I would like to thank my supervisor, Dr. Robert Jankov, for his wonderful guidance and support
throughout my project. His knowledge of neonatal medicine and beyond has been of
monumental importance, and I am truly grateful for his mentorship.
I would like to thank Dr. Patrick McNamara for sharing his expertise in 2D
echocardiography and Doppler ultrasound, and for his much appreciated participation as a
member of my supervisory committee. Also, I would like to thank Drs. Keith Tanswell and
Jacques Belik for providing invaluable insights into my project as members of my supervisory
committee.
To my laboratory colleagues, Julijana Damchevska and Crystal Kantores, my sincerest
gratitude, for making this experience even more enjoyable and rewarding. I would also like to
thank Ms. Rosetta Belcastro, Dr. Azhar Masood, Dr. Linda Li, Ms. Mandy Lau, Ms. Doreen
Engelberts, and Mr. Todd Van Vliet for their help and support.
Lastly, and importantly, I would like to thank my mother, Jingbai Nie, father, Huimin
Xu, brother, Richard Xu, and my friends for their love and support throughout this journey.
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TABLE OF CONTENTS
ABSTRACT ………………………………………………………………………… ii
ACKNOWLEDGEMENTS ………………………………………………………......... iii
TABLE OF CONTENTS …………………………………………………………........ iv
LIST OF FIGURES……….…………………………………………………………... vii
ABBREVIATIONS…….……………………………………………………………... ix
CHAPTER 1……………………………………………………………………......... 1
1. INTRODUCTION ………………………………………………………………… 2
1.1. GENERAL DESCRIPTION …………………..……………….............................. 2
1.2. FETAL TO NEWBORN VASCULAR TRANSITION …………………………...……. 4
1.3. DISEASE ETIOLOGY …………………………………………...…………….... 6
1.4. MOLECULAR TRIGGERS IN PHT DEVELOPMENT…………………….………… 7
1.4.1. RHOA/RHO-KINASE PATHWAY …………………………………...…... 10
1.4.2. NO-CGMP PATHWAY …………………………….…………………. 15
1.5. ROCK INHIBITORS AS A NOVEL TREATMENT FOR PHT ………………….…… 17
1.6. OTHER EXPERIMENTAL TREATMENTS FOR PHT ……………………………… 20
1.6.1. ET-1 RECEPTOR ANTAGONISTS………………………….……………. 20
1.6.2. TYPE V PHOSPHODIESTERASE (PDE-V) INHIBITORS………………...... 20
1.6.3. PLATELET-DERIVED GROWTH FACTOR (PDGF) RECEPTOR INHIBITORS.. 21
1.7. CHRONIC HYPOXIA MODEL OF NEONATAL PHT …………………...…………. 21
1.8. RATIONALE, GLOBAL AIMS, AND SPECIFIC HYPOTHESES ……………………... 23
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CHAPTER 2…………………………………………..…………………………….. 25
2. MATERIALS AND METHODS ……………..……………………………………… 26
2.1. MATERIALS …………………………………………………………………... 26
2.2. INSTITUTIONAL REVIEW …………………………………………………….... 27
2.3. HYPOXIA EXPOSURE SYSTEM ……………………………………………….... 28
2.4. INTERVENTIONAL STUDIES …………………………………………………… 28
2.5. TWO-DIMENSIONAL ECHOCARDIOGRAPHY & DOPPLER ULTRASOUND………... 29
2.5.1. PULMONARY VASCULAR RESISTANCE ……………………………….. 29
2.5.2. PULMONARY ARTERY SYSTOLIC PRESSURE ………………………….. 32
2.5.3. RIGHT VENTRICULAR OUTPUT …………………………...………… 32
2.6. EXAMINATION OF RIGHT VENTRICULAR HYPERTROPHY …………………….... 32
2.7. PERCENT MEDIAL WALL THICKNESS ………………………………………...... 33
2.8. IMMUNOHISTOCHEMISTRY ………………………………………………...…. 33
2.9. HART’S ELASTIN STAINING ………………………………………………….... 34
2.10. WESTERN BLOT ANALYSES ………………………………………………….... 35
2.11. PULMONARY ARTERY SMOOTH MUSCLE CELL (PASMC)-ENRICHED CULTURE. 36
2.12. TERMINAL DUTP NICK-END LABELLING (TUNEL) ASSAY …………………… 37
2.13. APOPTOSIS-DETECTION ELISA …………………………………………...….. 38
2.14. CELL VIABILITY ASSAY ………..…………………………………………..…. 39
2.15. DATA PRESENTATION AND ANALYSIS ……………………………………….... 39
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CHAPTER 3………………………...……………………………………………….. 40
3. RESULTS ………………………………………………………………….……. 41
3.1. BODY WEIGHT ………………………………………………………….…….. 41
3.2. PULMONARY VASCULAR RESISTANCE ………………………………………... 41
3.3. PULMONARY ARTERY SYSTOLIC PRESSURE …………………………………... 41
3.4. RIGHT VENTRICULAR PERFORMANCE …………………………………..…….. 45
3.5. RIGHT VENTRICULAR HYPERTROPHY ……………………………………... 45
3.6. ARTERIAL WALL REMODELLING …………………………………...…………. 45
3.7. PREPRO-ET-1 IMMUNOHISTOCHEMISTRY ……………………………..……… 50
3.8. PREPRO-ET-1 CONTENT ………..……………………………………..……… 50
3.9. ROCK-I AND ROCK-II CONTENT ….………………………………………… 50
3.10. MLC-2 PHOSPHORYLATION ……………………………………………..…… 50
3.11. PASMC PROLIFERATION …………………………………………………...… 56
3.12. KI-67 IMMUNOHISTOCHEMISTRY ………………………………………...…... 56
3.13. IN VITRO TUNEL AND ELISA ASSAY FOR APOPTOSIS ………………………... 56
3.14. IN VIVO TUNEL ASSAY ……………………………………………….……… 56
CHAPTER 4………………..……………………………………………………….. 62
4. DISCUSSION ……………………………………………………………..……... 63
4.1. LIMITATIONS AND FUTURE RESEARCH …………………………………...…… 66
5. REFERENCE LIST .…...………………………………………….……………... 69
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LIST OF FIGURES
CHAPTER 1
Figure 1 Fetal circulation ………………………………………………………….... 5
Figure 2 Progression from healthy to remodelled pulmonary vessels ……………… 7
Figure 3 Vasoconstriction pathway …………………………………………………. 8
Figure 4 The role of ROCK in calcium sensitisation, which results in smooth
muscle contraction ………………………………………………………… 10
Figure 5 Several mechanisms of ROCK activation and inactivation ……………….. 12
Figure 6 Smooth muscle contraction through activation of MAPK
by ROCK ………………………………………………………………….. 13
Figure 7 Smooth muscle contraction through activation of LIMK
by ROCK ………………………………………………………………….. 14
Figure 8 Smooth muscle contraction through activation of CPI-17 by PKC………... 15
Figure 9 Endogenous nitric oxide (NO) pathway …………………………………... 16
Figure 10 Molecular structures of Y-27632 and Fasudil …………………………….. 17
Figure 11 Actin immunostaining of pulmonary vessels ……………………………… 23
CHAPTER 2
Figure 12 Colour flow Doppler image of the pulmonary artery outflow tract ……... 30
Figure 13A Representative Doppler trace with pulmonary haemodynamic
measurements……………………………………………………..………... 30
Figure 13B Doppler trace of pulmonary artery outflow………………………….…….. 31
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CHAPTER 3
Figure 14 Body weights ……………………………………………………………… 42
Figure 15 Pulmonary vascular resistance (PVR) …………………………………….. 43
Figure 16 Pulmonary artery systolic pressure (PASP) …..…………………………… 44
Figure 17 Right ventricular performance ….…………………………………………. 46
Figure 18 Right ventricular hypertrophy (RVH) ……………………………………... 47
Figure 19 Percent medial wall thickness (% MWT) …………………………………. 48
Figure 20 Hart’s elastin stain ………………………………………………………….49
Figure 21 Prepro-ET-1 immunostaining ……………………………………………... 51
Figure 22 Prepro-ET-1 content ………..………………………………………………52
Figure 23 ROCK-I content ……….…………………………………………………... 53
Figure 24 ROCK-II content ….………………………………………………………. 54
Figure 25 Rho-kinase activity ………………………………………………………... 55
Figure 26 Proliferation index ………………………………………………………… 57
Figure 27 Immunohistochemical staining for Ki-67, a marker for DNA synthesis…... 58
Figure 28 Apoptosis in primary cultures of PASMC ………………………………… 59
Figure 29 Apoptosis index …………………………………………………………… 60
Figure 30 Apoptosis marker in frozen tissue sections ………………………………... 61
ix
ABBREVIATIONS
ANOVA Analysis of variance
Ca2+
Calcium ion
CaM Calmodulin
cGMP Cyclic guanosine monophosphate
CPI-17 Protein kinase C-potentiated myosin phosphatase inhibitor 17
ECMO Extracorporeal membrane oxygenation
ELISA Enzyme-linked immunosorbent assay
eNOS Endothelial nitric oxide synthase
ET-1 Endothelin-1
GAP Guanosine tri-phosphatase activating protein
GDI Guanine nucleotide dissociation inhibitors
GDP Guanine diphosphate
GEF Guanine nucleotide exchange factors
GTP Guanine triphosphate
IHC Immunohistochemistry
iNO Inhaled nitric oxide
LIMK Lin-II, Is1-1, and Mec-3 kinase
MAPK Mitogen-activated protein kinase
MLC-2 Myosin light chain
MLCK Myosin light chain kinase
MLCP Myosin light chain phosphatase
% MWT Percent medial wall thickness
x
NO Nitric oxide
NSAID Non-steroidal anti-inflammatory drug
O2•-
Superoxide radical
ONOO-
Peroxynitrite anion
PA Pulmonary artery
PAAT Pulmonary artery acceleration time
PASMC Pulmonary artery smooth muscle cell
PASP Pulmonary artery systolic pressure
PAVTI Pulmonary arterial velocity time integral
PDE-V Type 5 phosphodiesterase
PHT Pulmonary hypertension
PKA Protein kinase A
PKG Protein kinase G
PPHN Persistent pulmonary hypertension of the newborn
PVR Pulmonary vascular resistance
ROCK Rho-kinase
RV Right ventricle
RVET Right ventricular ejection time
RVH Right ventricular hypertrophy
RVI Right ventricular index
sGC Soluble guanylate cyclase
SMC Smooth muscle cell
TUNEL Terminal deoxynucleotidyl transferase d-uridine triphosphate nick end labelling
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1.1. General description
Pulmonary hypertension (PHT) is a debilitating disease characterised by an increase in
pulmonary arterial pressure and resistance. In early life, persistent pulmonary hypertension of
the newborn (PPHN) occurs in approximately 1 per 1000 term or near-term live births in North
America (Walsh-Sukys et al., 2000). PPHN usually presents within one to two days of birth,
and frequently results from clinical syndromes associated with persistent hypoxaemia, including
meconium aspiration and perinatal asphyxia (Evans & Archer, 1991; Walsh-Sukys, 1993;
Walsh-Sukys et al., 2000). Other conditions that may lead to PHT during the neonatal period
and infancy include congenital diaphragmatic hernia (Khemani et al., 2007; Mohseni-Bod &
Bohn, 2007; Soll, 2009) and severe cases of chronic lung disease of prematurity (Haworth,
1988; Rabinovitch, 1989; Thibeault et al., 2003; Parker et al., 2006). Persistent pulmonary
hypertension of the newborn has an associated mortality of 10-20% (Walsh-Sukys, 1993;
Walsh-Sukys et al., 2000) and survivors have an high morbidity (40-50%) in the form of
cognitive delays, cerebral palsy (Tanaka et al., 2007), hearing loss (Eriksen et al., 2009) and
frequent need for re-hospitalisation (Lipkin et al., 2002). The incidence of severe adverse
outcomes from other forms of neonatal PHT is likely higher.
An increased propensity to PHT in the newborn period, compared to other stages of life,
is predominantly related to two factors: (1) failure of the normal fall in pulmonary vascular
resistance (PVR) required for a successful transition to postnatal life and (2) the rapid
development and persistence of anatomical changes in the heart and pulmonary vasculature,
known collectively as “vascular remodelling”. Structural and functional consequences of
remodelling include narrowing of the vessel lumen, exaggerated responses to vasoconstrictors,
3
decreased relaxation and reduced responsiveness to vasodilators, all of which contribute to a
“fixed” increase in PVR. Increased PVR affects the right heart by increasing right ventricular
(RV) afterload, leading to right ventricular hypertrophy (RVH). Clinically, neonatal PHT
presents with an elevated FiO2 requirement and mechanical ventilation may be insufficient to
restore an adequate PaO2. If left untreated, right ventricular performance deteriorates, leading to
cor pulmonale and eventual death.
The current gold-standard treatment for neonatal PHT is inhaled nitric oxide (iNO),
which is approved for use in neonates above 35 weeks’ gestational age by Health Canada and
the United States Food and Drug Administration, and was the first therapy approved for
treatment of hypoxaemic respiratory failure following large clinical trials (NINOS, 1997;
Group, 1999; Clark et al., 2000; Clark et al., 2003; Li et al., 2009).
Though iNO is used extensively in NICUs across developed nations, there are a number
of serious drawbacks to its use, including non-responsiveness in up to 40% of patients. For
those patients who responded initially, rebound PHT (upon attempted weaning from iNO) or
non-sustained response is frequently observed. Rebound PHT is thought to be caused by a
down-regulation of endogenous NO production (Lee et al., 2008) and/or upregulated type 5
phosphodiesterase (PDE-V) expression following iNO treatment (Namachivayam et al., 2006).
Though most patients respond to iNO therapy in terms of improved systemic oxygenation and a
decreased need for more invasive interventions, such as extracorporeal membrane oxygenation
(ECMO), its use has not been associated with improvements in long term outcomes such as
cerebral palsy (NINOS, 2000; Clark et al., 2003), or in overall mortality rates (NINOS, 1997).
Furthermore, due to the high cost and the sophisticated equipment required for administration,
iNO is largely unavailable in developing nations. Currently, the usual second-line option for
4
neonates who do not respond to iNO is ECMO, which has been shown to decrease mortality
(Fakioglu et al., 2005), though it is associated with substantial risks of intracranial haemorrhage,
further contributing to neurocognitive impairment later in life (Short, 2005). Thus, the
investigation of novel treatments for PPHN patients who are nonresponsive to current
conventional therapies remains a high priority, and is the focus of this thesis.
1.2. Fetal-to-newborn vascular transition
All newborns must undergo a dramatic shift in circulation patterns in order to
successfully transition from an environment within the womb to the outside world. During fetal
life, less than 10% of the combined ventricular output passes through the lungs; the rest of the
outflow from the right ventricle passes through the patent foramen ovale or ductus arteriosus to
the systemic circulation (Fig. 1). These pathways are maintained because of the high resistance
in pulmonary arteries (PAs). The high resistance, in turn, is due to constriction of the relatively
abundant, muscular-walled, PAs. Transition from fetal to newborn circulation involves
elimination of the placental circulation, transfer of the function of gas exchange from the
placenta to the lungs, and closure of the fetal pulmonary-systemic shunts. A marked fall in
pulmonary vascular resistance (PVR), resulting in a dramatically increased pulmonary blood
flow, is central to this transition. The low-impedance placenta is lost at birth, and as a result,
high systemic and low PVR characterises the neonatal circulation. The fall in PVR occurs in
two phases. The first phase, commencing immediately after birth, is marked by a dramatic
decrease in pulmonary arterial tone, and therefore a dilatation of pulmonary vessels. Factors that
contribute to this phenomenon include expansion of the lungs with air after birth and the higher
oxygen tension of ambient air. The second, and more gradual, phase is associated with a
5
decrease in the muscularisation of arterial walls and a resultant relative increase in the number
of non-muscularised pulmonary arteries. A failure of the normal postnatal decrease in PVR
characterises PPHN, which presents as persistent cyanosis and hypoxaemia with or without
cardiac dysfunction.
Figure 1. Fetal circulation. The placenta oxygenates blood for the growing fetus, to which it
flows from the umbilical vein through the ductus venosus to the inferior vena cava, the right
atrium, the right ventricle, and is then pumped into the pulmonary artery. Due to high
pulmonary vascular resistance and an open ductus arteriosus, the majority of blood flow is from
the pulmonary artery through the ductus arteriosus and into the aorta; blood also flows across
the foramen ovale from the right to the left atria. Reproduced from the website of Lucile
Packard Children’s Hospital in Stanford:
http://www.lpch.org/DiseaseHealthInfo/HealthLibrary/hrnewborn/0181-pop.html.
6
The second phase, largely complete by two months of postnatal age, is dependent upon
the maintenance of low PVR. A reduction in the weight of the right ventricle relative to the left,
and a decrease in wall thickness of the major pulmonary arteries accompany this change in the
pulmonary arteries. Right ventricular weight is closely related to pulmonary arterial muscle
mass in vessels of varying sizes, making the presence of a relative hypertrophy of the right
ventricle a useful marker of PHT (Rabinovitch et al., 1979).
1.3. Disease etiology
Pulmonary hypertension presenting in early life results from one or more of the
following pathophysiological mechanisms: underdevelopment, maldevelopment, or
maladaptation of the pulmonary vasculature.
In cases of underdeveloped pulmonary vasculature, raised PVR is relatively permanent,
and is found in a variety of conditions, including congenital diaphragmatic hernia, cystic
adenomatoid malformation of the lung, and pulmonary hypoplasia syndromes. Because of the
relative permanence of PHT due to underdevelopment, patients who possess these conditions
tend to be the most difficult to treat and have the worst outcomes (Levin, 1978).
Maldevelopment of the pulmonary vasculature results from abnormalities involving
bronchiolar branching and alveolar differentiation, the number of pulmonary vessels in the
lungs, and/or an increase in the muscularisation of the pulmonary vessels, especially into the
typically non-muscularised intra-acinar vessels of the pulmonary system (Murphy et al., 1981),
leading to failure of normal pulmonary arterial relaxation after birth. Additionally, it has been
shown that some drugs taken by the mother during gestation may induce maldevelopment of the
pulmonary vasculature in newborns, resulting in an increased incidence of PPHN (Belik, 2008).
7
These drugs include non-steroidal anti-inflammatory drugs (NSAIDs) (eg: indomethacin,
ibuprofen) and the anti-depressant drugs of the serotonin reuptake-inhibitor class (SRIs) (eg:
Prozac, Zoloft, Paxil), which have been shown to increase the incidence of PHT, evidenced by
remodelling of the pulmonary vasculature (Alano et al., 2001; Chambers et al., 2006; Belik,
2008).
Lastly, PHT may result from maladaptation of a fetal pulmonary vascular bed that is ill-
equipped to adapt to extrauterine life. Maladaptation is known to result from such conditions as
perinatal asphyxia, pulmonary parenchymal diseases (meconium aspiration, congenital
pneumonia), and congenital sepsis (Curtis et al., 2003; Dakshinamurti, 2005).
1.4. Molecular triggers in PHT development
Increased PVR is related to two phenomena: (1) sustained vasoconstriction and (2)
vascular remodelling, the latter being the pathological hallmark of PHT in neonates and children
(Fig. 2).
Figure 2. Progression from a healthy to a remodelled pulmonary vessel. Reproduced with the
permission of Dr. A. Keith Tanswell.
8
Vascular remodelling is characterised by the muscularisation of normally non-
muscularised pulmonary vessels, such as intra-acinar PAs, and the hyperplasia and hypertrophy
of medial wall smooth muscle cells (SMCs) in arteries that are normally muscularised (Kantores
et al., 2006). Once established, remodelling has traditionally been believed to be non-reversible,
contributing to poor responses to current therapies and to an increased potential for a
progressive worsening of the PHT and eventual death (Guilluy et al., 2009). Thus, it is
important to understand how this process occurs, and the mechanisms underlying the
development and persistence of sustained vasoconstriction and remodelling of the pulmonary
vasculature during the neonatal period.
A major cellular mechanism of pulmonary vasoconstriction involves the activation of G-
proteins, which are located at the plasma membranes of smooth muscle cells surrounding
pulmonary arterioles (Fig. 3).
Figure 3. Vasoconstriction pathway. Ca2+
= calcium ions, CaM= calmodulin, MLC-2= myosin
regulatory light chain, MLCK= myosin light chain kinase, MLCP= myosin light chain
phosphatase, P= phosphate molecule.
9
G-proteins are activated by hypoxia and binding of G-protein-coupled receptor (GPCR)
ligands, such as endothelin-1 (ET-1) and thromboxane A2. Activated G-proteins open calcium
ion (Ca2+
) channels at the plasma membrane and at the sarcoplasmic reticulum membranes
within the cell, allowing the entry of Ca2+
into the cell, and the release of sequestered Ca2+
from
stores in the endoplasmic reticulum, respectively. Calcium then binds to calmodulin, creating
the Ca2+
-calmodulin complex (Ca2+
-CaM). Ca2+
-CaM activates myosin light chain kinase
(MLCK), which in turn, phosphorylates myosin light chain (MLC-2, also known as MLC, LC-
20, or MRSLC), resulting in increased smooth muscle contraction. Conversely, the enzyme
myosin light chain phosphatase (MLCP) is involved in the dephosphorylation of MLC-2,
leading to smooth muscle relaxation.
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1.4. 1. RhoA/Rho-kinase pathway
Another mechanism whereby sustained vasoconstriction may occur is through a pathway
involving a phenomenon known as “calcium sensitisation” (Fig. 4).
Figure 4. The role of ROCK in calcium sensitisation, which contributes to sustained smooth
muscle contraction. GDP= guanosine diphosphate, GTP= guanosine triphosphate, MLC-2=
myosin light chain, MLCK= myosin light chain kinase, MLCP= myosin light chain phosphatase,
RhoA= Rho GTP family of proteins, member A, ROCK= rho-kinase.
This phenomenon generally results when an increase in smooth muscle cell contraction occurs
without a change in Ca2+
concentration, and is thought to be mainly due to the phosphorylation
and deactivation of the enzyme MLCP. Phosphorylated MLCP is not able to dephosphorylate
MLC-2, and muscle contraction persists. This activity is mediated through the actions of a
small protein in the Rho GTP family of proteins, RhoA, and its effector protein, Rho-kinase
(ROCK) (Somlyo et al., 1999). ROCK has two known isoforms, ROCK-I (ROCK-β) and
11
ROCK-II (ROCK-α) and both are found ubiquitously throughout the vasculature (Nakagawa et
al., 1996).
Rho GTP binding proteins consist of a large number of Rho, Rac, and Cdc42 subfamilies
that are involved in many cellular processes such as gene transcription, differentiation,
proliferation, hypertrophy, apoptosis, phagocytosis, adhesion, migration, and contraction
(Riento & Ridley, 2003; Jaffe & Hall, 2005). Moreover, there are many molecules involved in
both the activation and deactivation of ROCK, such as guanine nucleotide exchange factors,
guanine nucleotide disassociation inhibitors, and GTPase-activating proteins, among others.
Cellular mechanisms leading to the activation of ROCK are believed to begin with
activation of G-proteins at the smooth muscle cell membrane. This activates GEFs, leading to
replacement of GDP by GTP on the RhoA GTPase (Fig. 5). RhoA-GTPase translocates to the
cell membrane, activating a number of downstream effectors, including ROCK. ROCK can
become deactivated by a series of negative regulators such as: GDIs that inhibit the exchange of
GDP by GTP; GAPs that convert RhoA-GTP to RhoA-GDP; statins that inhibit the
translocation of RhoA-GTP to the cell membrane; and protein kinases A (PKA) and G (PKG)
which also prevent translocation of RhoA-GTP to the cell membrane (Sawada et al., 2001;
Murthy, 2006).
12
Figure 5. Several mechanisms of ROCK activation and inactivation. GAP= GTPase activating
proteins, GDI= guanine nucleotide dissociation inhibitors, GDP= guanylate diphosphate,
GEF= guanine nucleotide exchange factors, GTP= guanylate triphosphate, PKA= protein
kinase A, PKG= protein kinase G.
The role of ROCK in the development of PHT has recently become an issue of
considerable interest, as it is now believed that ROCK may play a central role in the regulation
of vasoconstriction. This belief has evolved from an increased appreciation of the influence of a
number of physiological (eg: hypoxia) or biochemical (eg: serotonin; mitogen-activated protein
kinase- MAPK; Lin-II, Is1-1, and Mec-3 kinases- LIMK; nitric oxide, reactive oxygen species,
and endothelin-1) factors on ROCK, many of which are believed to contribute to the
pathogenesis of PHT (McMurtry et al., 2003).
Recently, RhoA was demonstrated to respond to the transport of serotonin (5-HT)
through the cell membrane of pulmonary artery smooth muscle cells (PASMCs) via serotonin
transporters (5-HTT) (Guilluy et al., 2009). The transport of 5-HT from outside of the cell into
the cell was demonstrated to result in RhoA serotonylation, which in turn resulted in increased
ROCK activity in the lungs, platelets, and PASMCs of patients with PHT (Guilluy et al., 2009).
13
ROCK is also known to regulate the expression of mitogen-activated protein kinase (p38
MAPK), Lin-II, Is1-1, and Mec-3 kinases (LIMK), and protein-kinase C-potentiated myosin
phosphatase inhibitor (CPI-17), all of which are known effectors of SMC contraction.
MAPK regulates smooth muscle contraction and, when activated by ROCK (Fig. 6),
phosphorylates heat shock protein 27 (HSP27) (Lopez-Ilasaca, 1998; Nwariaku et al., 2003;
Galaria et al., 2004). This activates HSP27, leading to increased polyermized actin stabilisation,
which leads to increased muscle contraction (Yamboliev et al., 2000).
Figure 6. Smooth muscle contraction through activation of MAPK by ROCK. HSP27= heat
shock protein 27, MAPK= mitogen-activated protein kinase, ROCK= Rho-kinase.
ROCK also affects the enzyme LIMK (Fig. 7). ROCK phosphorylates LIMK, which
then phosphorylates an actin-binding protein called cofilin, leading to its inactivation (Maekawa
et al., 1999). Inactivation of cofilin contributes to actin polymerization and thereby enhanced
potential for vasoconstriction (Sakamoto et al., 2003). Sakamoto et al. (2003) and Somlyo and
Somlyo (2003) have demonstrated that Y-27632 inhibited LIMK phosphorylation, which led to
a decrease in vaso-reactivity as well as a disruption in the actin cytoskeleton, which eventually
resulted in an attenuation of LIMK-related vasoconstriction.
14
Figure 7. Smooth muscle contraction through activation of LIMK by ROCK. LIMK= Lin-II,
Is1-1, and Mec-3 kinase, ROCK= Rho-kinase.
It is believed that CPI-17 is also affected indirectly by ROCK (Fig. 8). CPI-17 is
phosphorylated by protein kinase C (PKC), and when phosphorylated, CPI-17 inhibits the
activity of MLCP, leading to persistent vasoconstriction (Sakai, 2004). It has been shown that
ROCK inhibition has resulted in decreased CPI-17 phosphorylation, and thus attenuation of
SMC contraction (Sakai, 2004; Pourmahram et al., 2008).
15
Figure 8. Smooth muscle contraction through activation of CPI-17 by PKC. CPI-17= protein-
kinase C-potentiated myosin phosphatase inhibitor, MLC-2= myosin light chain, MLCK=
myosin light chain kinase, MLCP= myosin light chain phosphatase, PKC= protein kinase C,
ROCK= Rho-kinase.
1.4. 2. NO-cGMP pathway
Another major regulator of pulmonary vascular tone is the nitric oxide-cyclic guanosine
monophosphate (NO-cGMP) pathway. Nitric oxide is produced from L-arginine in endothelial
cells through the activity of the enzyme endothelial nitric oxide synthase (eNOS) (Fig. 9).
Nitric oxide diffuses into smooth muscle and acts upon its intracellular receptor, soluble
guanylate cyclase (sGC). Activation of sGC leads to increased production of cyclic guanosine
monophosphate (cGMP), which causes Ca2+
desensitisation and relaxation of smooth muscle via
increased activity of PKG.
16
Figure 9. Endogenous nitric oxide (NO) pathway. 5’-GMP= 5’- guanylate monophosphate,
cGMP= cyclic guanylate monophosphate, eNOS= endothelial NO synthase, GTP=guanine
triphosphate, NO= nitric oxide, PDE V= type 5 phosphodiesterase, PKG= protein kinase G,
sGC= soluble guanylate cyclase.
The bioavailability of NO may be directly affected by the oxygen radical superoxide
(O2•-), through the formation of NO into the peroxynitrite anion (ONOO
-), which may itself
contribute to the pathogenesis of PHT (Jankov et al., 2000; Belik et al., 2004; Abman, 2007).
Furthermore, low concentrations of L-arginine, a NO precursor, oxidisation of sGC and an
increase in activity of PDE-V (a cGMP-degrading enzyme), are also likely to further contribute
to PHT (Pearson et al., 2001; Andersen et al., 2008). The likelihood of reciprocal interactions
between the RhoA/ROCK and NO-cGMP pathways is evidenced by the following: reports of
the inhibitory effects of PKG on RhoA activation (Sawada et al., 2001; Murthy, 2006); the
decreased expression of endothelin-1 (ET-1), a major upstream effector of ROCK, in response
to stimulation of cGMP-mediated pathways (Kourembanas et al., 1993); and the down-
regulation of eNOS expression resulting from increased ROCK activity (Abe et al., 2006).
Therefore, the enhanced activity of one pathway appears to lead to the diminished activity of the
other.
17
1.5. ROCK inhibitors as a novel treatment for PHT
Two pharmacological Rho-kinase inhibitors, Y-27632 (Ishizaki et al., 2000) and Fasudil
(HA-1077) (Sasaki et al., 2002) (Fig. 10), though structurally dissimilar, have both been shown
to possess high specificity toward the two known ROCK isoforms (ROCK-I and ROCK-II)
when compared to a broad range of other kinases (Davies et al., 2000). This specificity has led
to the recognition that the activation of ROCK may be a central convergence point for multiple
pathways that can induce both sustained vasoconstriction and remodelling of pulmonary
resistance arteries.
Figure 10. Molecular structures of Y-27632 and Fasudil (HA-1077).
An increased appreciation of the importance of vascular remodelling in the pathogenesis
of chronic PHT has led to a shift in focus away from drugs that act solely as pulmonary
vasodilators, towards treatments that target and attenuate PASMC hyperplasia through pro-
apoptotic and/or anti-proliferative effects. Although patients with PHT have increased vascular
muscularisation, along with persistent pulmonary vasoconstriction, current treatments
(particularly iNO) target their role as vasodilators. However, once vascular remodelling is
18
established, such therapies are less likely to be efficacious (Guilluy et al., 2009). Drugs that
dilate pulmonary vessels and have pro-apoptotic/anti-proliferative effects on vascular wall
SMC’s, would be more likely to reverse chronic PHT. Rho-kinase inhibitors, such as Y-27632
and Fasudil, are unique in having been shown to both dilate the remodelled pulmonary
vasculature and to promote apoptosis in various cell types, thus providing a strong rationale for
the potential use of ROCK inhibitors as a treatment for chronic PHT.
Y-27632, the ROCK inhibitor used in experiments contributing to this thesis has been
shown to have a 50% lower IC50 on ROCK activity than Fasudil, and has been used in adult
animal models of PHT with beneficial attenuating affects on structural changes of PHT
(Doggrell, 2005; Rattan & Patel, 2008). Y-27632 (Fig.10) is a serine-threonine ROCK inhibitor
that competitively binds to ATP binding sites on the ROCK enzyme (Doggrell, 2005), and has
been shown to have vasodilatory effects in many different studies. ROCK inhibitors have been
reported to inhibit pulmonary artery myogenic responses in hypoxia-exposed adult rats
(Broughton et al., 2008) and fetal sheep (Tourneux et al., 2008) and to reverse sustained
pulmonary vasoconstriction in response to hypoxia (Fagan et al., 2004; McNamara et al., 2008),
bleomycin (McNamara et al., 2008) or the infusion of vasoconstrictors, such as endothelin-1
(Weigand et al., 2006). When delivered directly to the lung, Y-27632 was found to acutely
decrease PVR in adult rats with PHT induced by hypoxia (Nagaoka et al., 2005).
In cultured PASMCs, treatment with Y-27632 resulted in decreased formation of stress
fibres and attenuated Ca2+
sensitisation (Uehata et al., 1997). Chen reported attenuating effects
of ROCK inhibitors on PASMC proliferation induced by 5-HT (Chen et al., 2009). Such results
may help explain the effects of chronic treatment with ROCK inhibitors in preventing the
structural changes of PHT in adult rodent models. Systemic administration of ROCK inhibitors,
19
commenced at the onset of injury, has been reported to prevent vascular remodelling induced
either by hypoxia (Fagan et al., 2004) or monocrotaline (Abe et al., 2004). Y-27632 also
enhanced eNOS expression and resulted in the attenuation of chronic hypoxia-induced
angiogenesis (Fagan et al., 2004; Hyvelin et al., 2005). Furthermore, in monocrotaline-exposed
adult rats, a ROCK inhibitor was reported to prevent progression of disease leading to mortality
and to induce regression of vascular remodelling when commenced after the injury was already
well established (Abe et al., 2004).
Several pilot studies examining the effects of a single bolus dose of ROCK inhibitor
(Fasudil) have been published, demonstrating that intravenous Fasudil administered to adult
humans with idiopathic chronic PHT (Nagaoka et al., 2005; Ishikura et al., 2006) and children
with congenital heart disease-associated PHT (Li et al., 2009) lowered PA pressure and PVR.
Subsequent studies have shown the RhoA and ROCK pathway to be activated in pulmonary
vessels of adult humans with PHT (Do e et al., 2009; Guilluy et al., 2009).
Though there were significant benefits to the use of ROCK inhibitors for treatment of
PHT in both experimental models and humans, no improvements in right ventricular
performance have yet been described. This is an important factor to consider, as decreased right
ventricular performance is an important prognostic factor for PHT: its presence being highly
predictive of adverse outcome (McNamara et al., 2008; Bogaard et al., 2009).
20
1.6. Other experimental treatments for PHT
1.6.1. ET-1 receptor antagonists
ET-1 is an important vasoconstrictor that affects many pathways leading to PHT. ET-1
has two receptors, ETA and ETB; ETA is known to increase vasoconstriction and proliferation of
vascular SMCs and ETB is thought to be involved in ET-1 degradation, and therefore
contributing to clearance of circulating ET-1. The activation of ETB has been shown to result in
vasodilatation and NO release (Badesch et al., 2004). Bosentan (Tracleer®), an antagonist of
both ETA and ETB receptors, received Health Canada approval in 2001 for the treatment of
chronic PHT in adults (Michelakis et al., 2002). Clinical experience with Bosentan in newborns
is limited, partly related to potential concerns regarding hepatic toxicity (Zhao et al., 2001;
Michelakis et al., 2002). Expression of prepro-ET-1, a precursor to ET-1, was examined in this
thesis.
1.6.2. Type V phosphodiesterase (PDE-V) inhibitors
PDE-V is involved in the endogenous NO pathway (Fig. 9), by degrading cGMP,
resulting in smooth muscle cell contraction. PDE-V inhibitors, such as Sildenafil, have been
shown to improve PHT pathology by decreasing the rate of degradation of cGMP, resulting in
smooth muscle cell relaxation (Zhao et al., 2001; Lee et al., 2008). Based on the literature,
PDE-V inhibitors show promise as an adjunct treatment for neonatal PHT as well as a treatment
administered following NO weaning to decrease risks of rebound PHT (Galie et al., 2005;
Namachivayam et al., 2006; Lee et al., 2008), though experience with PHT in newborns is
currently limited to clinical trials.
21
1.6.3. Platelet-derived growth factor (PDGF) receptor inhibitors
PDGFs act as mitogens affecting the growth and development as well as the migration of
SMCs and fibroblast cells (Ostman et al., 1992; Haniu et al., 1993; Haniu et al., 1994). PDGFs
exist in five dimeric isoforms: PDGF-AA, PDGF-AB, PDGF-BB, PDGF-CC and PDGF-DD
(Haniu et al., 1994). PDGF isoforms can bind to two different receptors, PDGF-α receptor
(PDGF-αR) and PDGF-β receptor (PDGF-βR) (Dalla-Favera et al., 1982). These receptors have
been found to be upregulated in lambs with chronic intrauterine pulmonary hypertension when
compared with control animals (Balasubramaniam et al., 2003). Furthermore, it was
demonstrated that human cases of severe pulmonary arterial hypertension exhibited an
overexpression of PDGF-AA (Humbert et al., 1998). Given the increasing evidence that one or
more PDGFs may play a role in the pathogenesis of vascular remodelling, there has been
interest in the use of drugs which antagonize this pathway. Tyrosine kinase inhibitors such as
imatinib mesylate, have been shown to reverse remodelling in adult models, have shown
therapeutic promise in experimental models of chronic PHT in which vascular SMC apoptosis
was increased (Schermuly et al., 2005; Chhina et al., 2010).
1.7. Chronic hypoxia model of neonatal PHT
Rodents are highly suitable as models for neonatal lung injury, given that alveolar and
acinar (distal airway-associated) vascular development are postnatal events (Burri, 1974) that
share many similarities with human neonatal PHT. Rats are the preferred species for modeling
PHT, as injury develops much more readily in rats than in mice (Rabinovitch et al., 1981; Chen
et al., 2006). Experimental studies in the immature rat have demonstrated a unique
susceptibility, when compared to adults, to the development of a rapidly progressive form of
22
pulmonary vasculopathy, characterised by severe vascular remodelling and cardiac dysfunction
(Rabinovitch et al., 1981; Kantores et al., 2006; McNamara et al., 2008), ultimately leading to
death. In humans with neonatal PHT, abnormalities in pulmonary vascular function have been
described to persist into adulthood (Sartori et al., 1999). Similarly, recovery from pulmonary
vascular injury in the immature rat is likely to be delayed and incomplete (Rabinovitch et al.,
1981; King et al., 1995; Keith et al., 2000), contributing to impaired lung growth (Meyrick &
Reid, 1981, 1982; Fabris et al., 2001) and a high potential for recurrence of PHT in later life
(Hampl & Herget, 1990; Caslin et al., 1991; King et al., 1995).
With the goal of testing novel approaches to therapy, our laboratory has developed a
neonatal Sprague Dawley (SD) rat model of chronic hypoxic PHT secondary to exposure to
13% O2 from birth until 14 days of life (Kantores et al., 2006). Pathological features of PHT in
this model include structural (RV hypertrophy and arterial medial wall thickening; Fig. 11) and
functional (increased PVR and RV dysfunction) abnormalities. Furthermore, once chronic PHT
is established (by 14 days), this injury model is unresponsive to iNO (McNamara et al., 2008),
replicating the “fixed” and often-fatal form of human neonatal PHT.
23
Figure 11. Actin immunostaining of pulmonary vessels. Note the increased expression of actin
(dark brown), a marker for smooth muscle, in lung sections from a chronic hypoxia-exposed
pup, compared to sections from a normoxia-exposed pup; Hematoxylin (light blue) stains all cell
nuclei. Arrows point to pulmonary vessels.
1.8. Rationale, global aims and specific hypotheses
We have previously shown that the RhoA/ROCK pathway is activated in the pulmonary
vasculature of SD rat pups with chronic PHT induced by exposure to 13% O2 from birth to 14
days (McNamara et al., 2008). In acute studies using this model, a single bolus of the ROCK
inhibitor, Y-27632, had far superior vasodilatory effects upon the hypertensive pulmonary
circulation when compared to the current “gold standard” therapy, iNO (McNamara et al.,
2008). Furthermore, we have shown that treatment with Y-27632 from birth, concurrent with
hypoxia exposure, prevented vascular remodelling through inhibitory effects on arterial wall
smooth muscle cell proliferation (Ziino et al., 2010). These studies indicate that ROCK is
critical to sustained vasoconstriction and mediates smooth muscle proliferation and arterial wall
remodelling in the chronic hypoxia-exposed neonatal rat.
24
Based upon these findings, the global aim of the studies upon which this thesis is based
was to determine whether late sustained (or “rescue”) treatment with Y-27632 (from day 14-21
of life), commenced after chronic PHT was already established, would reverse the structural and
functional changes of chronic hypoxic PHT. Reversal of the pathological changes of chronic
PHT is an important therapeutic goal, as the continued presence of these changes may increase
the likelihood of progression toward fatal PHT in later life (Hampl & Herget, 1990; Caslin et
al., 1991).
Specifically, my hypotheses were that late-sustained treatment with the ROCK inhibitor,
Y-27632, in neonatal rats with established chronic hypoxic PHT would:
1. normalise raised PVR and RV dysfunction
2. reverse structural abnormalities, including RVH and arterial medial wall thickening, and
lead to inhibited proliferation and augmented apoptosis of pulmonary arterial smooth
muscle cells
26
2.1. Materials
The Rho-kinase inhibitor, Y-27632, was purchased from Alexis Biochemicals (San
Diego, CA, U.S.A.). Oxygen exposure chambers and automated controllers (OxyCycler model
A84XOV) were from Biospherix (Redfield, NY, U.S.A.). Phos-tag acrylamide was purchased
from NARD Institute (Amagasaki City, Hyogo, Japan). Total protein assay kits, tris-glycine
gels and poly-vinylidene difluoride (PVDF) membranes were from BioRad (San Diego, CA,
U.S.A.). Protease inhibitors, Cell Death Detection ELISAPLUS
and terminal deoxyuridine
triphosphate (dUTP) nick-end labelling (TUNEL) assay kits were purchased from Roche (Laval,
QC, Canada). Dulbecco’s modified Eagle’s medium (DMEM), antibiotic-antimycotic solution,
trypsin and ethylenediamine tetra-acetic acid (EDTA) were from Gibco BRL (Burlington, ON,
Canada). Heat-inactivated fetal bovine serum (FBS) and normal goat serum (NGS) were from
Flow Laboratories (McLean, VA, U.S.A.); collagenase and DNAse were from Worthington
(Freehold, NJ, U.S.A.). Acids, alcohols, chromatography-grade organic solvents, H2O2,
Permount and Superfrost/Plus microscope slides were purchased from Fisher Scientific
(Markham, ON, Canada). All other chemicals and reagents were purchased from Sigma
Chemical Co. (Oakville, ON, Canada).
Goat anti-rabbit and anti-mouse immunoglobulin (IgG)-peroxidase antibodies were from
Cell Signaling Technology (Beverly, MA). Goat anti-rabbit, goat anti-mouse and donkey anti-
goat IgG-biotin antibodies were from Santa Cruz Biotechnology (Santa Cruz, CA, U.S.A.). 6-
diamino-2´-phenylindole (DAPI) mounting medium, and 3, 3´ diaminobenzidine (DAB)
staining kits were from Vector Laboratories (Burlingame, CA, U.S.A.). Aqueous mounting
medium was from DAKO Cytomation (Carpenteria, CA, U.S.A.). Wst-8 Cell Proliferation kits
27
were from Cayman Chemical Co. (Ann Arbor, MI, U.S.A.). Primary antibody sources and
concentrations used for Western blot (WB) and/or immunohistochemistry (IHC) on paraffin-
embedded tissue are as follows:
Antibody (Source) WB IHC Catalogue #
α-Smooth muscle actin 1:5000 1:1000 MS-113-PI
(Neomarkers, Fremont, CA, U.S.A.)
Glyceraldehyde-3-phosphate dehydrogenase 1:5000 ---------- SC-25778
(Santa Cruz Biotechnology, Santa Cruz, CA, U.S.A.)
Myosin Regulatory Light Chain 1:2000 ---------- SC-15370
(Santa Cruz Biotechnology, Santa Cruz, CA, U.S.A.)
Rho-kinase I (Santa Cruz, CA, U.S.A.) 1:2000 ---------- SC-17794
Rho-kinase II (Santa Cruz, CA, U.S.A.) 1:200 ---------- SC-5561
Ki67 antigen (Dako, Carpenteria, CA, U.S.A.) ---------- 1:25 M-7248
Prepro-endothelin-1 ---------- 1:200 T-4306.0050
(Cedarlane, Burlington, ON, Canada)
Prepro-endothelin-1 1:3000 ---------- MA3-005
(Thermo Scientific, Rockford, IL, U.S.A.)
2.2. Institutional review
All procedures involving animals were conducted according to criteria established by the
Canadian Council on Animal Care. Approval for studies was obtained from the Sunnybrook
Research Institute Animal Care Committee.
28
2.3. Hypoxia exposure system
Pathogen-free timed pregnant SD rats were obtained from Taconic (Germantown, NY,
U.S.A.). Experiments were conducted as paired exposures with one litter receiving 13% O2
(hypoxia) and another litter receiving 21% O2 (air) from day one of life for up to 17 or 21 days,
depending upon the endpoint of interest. O2 and CO2 concentrations, temperature and humidity
were continuously monitored, recorded, and regulated by computer using customised software
(AnaWin2 Run-Time, version 2.2.18, Watlow-Anafaze, St. Louis, MO, U.S.A.). Gas delivery
was automatically adjusted to maintain an O2 concentration within 0.1% of the set point. O2
sensors were calibrated weekly. On the anticipated day of delivery, each dam was placed in an
100 × 80 × 60 cm Plexiglass chamber with 12 h/12 h light-dark cycles, and with temperature
maintained at 25 ± 1°C, humidity ≈ 50%, and CO2 concentration <0.5%. Equal litter sizes (10-
12 pups) and sex distribution were maintained throughout the exposure period. Food and water
were available ad libitum. Dams were exchanged daily between paired air and hypoxia
chambers to prevent any maternal toxicity and consequent nutritional effects on the pups. At
the end of each exposure period, pups were either killed by exsanguination after anaesthesia or
by pentobarbital sodium overdose.
2.4. Interventional studies
Injections (15 mg/kg body weight) were given subcutaneously (s.c.) via a 30-gauge
needle twice per day (bis in die or b.i.d.) for a daily dose of 30 mg/kg body weight) starting on
postnatal day 14.
29
2.5. Two-dimensional echocardiography and Doppler ultrasound
Two-dimensional echocardiography and Doppler ultrasound, performed by Dr.
McNamara, was employed as a non-invasive method for assessment of pulmonary
haemodynamics using a Vivid 7 Advantage cardiovascular ultrasound system (GE Medical
Systems, Milwaukee, WI) with a small high frequency linear probe (I13L).
An ultra-high frame
rate provided high image quality, which was found to be particularly suitable for small animal
imaging, in which the heart rate is very rapid. Immediately following administration of
anesthesia with intraperitoneal (i.p.) ketamine hydrochloride (40 mg/kg) and xylazine
hydrochloride (6 mg/kg), the animal was laid supine and the probe was gently applied to the
chest while the animal was spontaneously breathing room air. For measurements of pulmonary
arterial haemodynamics, a short axis view at the level of the aortic valve was obtained, and the
pulmonary artery was identified using colour flow Doppler (Fig. 12). Analysis was undertaken
in a blinded fashion.
2.5.1. Pulmonary vascular resistance
Pulmonary vascular resistance is widely used as a marker for severity of pulmonary
hypertension (Ananthakrishnan et al., 2009; Corte et al., 2009; Rame, 2009). The pulsed
Doppler gate was placed proximal to the pulmonary valve leaflets and aligned, with an angle of
insonation < 20°, to maximize laminar flow. The pulmonary artery acceleration time (PAAT)
and right ventricular ejection time (RVET) were then estimated using the pulmonary Doppler
profile (Figs. 13A and 13B). PAAT was measured as the time from the onset of systolic flow to
peak pulmonary outflow velocity, and RVET was measured as the time from onset to
30
completion of systolic pulmonary flow. A surrogate measure of PVR was calculated according
to the formula: PVR= 1/ (PAAT: RVET) (Jones et al., 2002).
Figure 12. Colour flow Doppler image of the pulmonary artery outflow tract, used to derive
measurements of pulmonary vascular resistance and right ventricular output. Blue colour
represents blood flow away from the echo probe.
Figure 13A. Representative Doppler trace used to obtain measurements of pulmonary
haemodynamic. PAAT= pulmonary artery acceleration tract, RVET=right ventricular ejection
time, and PAVTI (area under the curve)= pulmonary arterial velocity time integral. Arrow
highlights mid-systolic “notching” pattern often seen in severe PHT.
31
Figure 13B. Doppler trace of pulmonary artery outflow. Note differences in shape of traces in
the untreated hypoxia control (top) and the Y-27632-treated hypoxia animals (bottom). Used
with permission from the American Physiological Society (McNamara et al., 2008).
32
2.5.2. Pulmonary artery systolic pressure
An estimation of pulmonary artery systolic pressure (PASP) was derived from the
PAAT, using the formula PASP=137.2 -3.3 x PAAT (Jones et al., 2002).
2.5.3. Right ventricular output
Right ventricular output was used as an index of RV performance, which is decreased in
severe pulmonary hypertension (Hoeper et al., 2001; Liu et al., 2009). The diameter of the
pulmonary artery (PAD) was measured by colour flow Doppler at the hinge-point of the
pulmonary valve leaflets. From the same Doppler interrogation of the pulmonary artery used to
measure PAAT and RVET, right ventricular stroke volume was estimated using the formula:
(PAD/2)2 x 3.14 x pulmonary artery velocity time integral (PAVTI). PAVTI was measured by
tracing the leading edge of the velocity time graph from the onset to completion of systolic
pulmonary flow. Right ventricular stroke volume was corrected for heart rate and body weight
to derive a right ventricular index (RVI). (Hoeper et al., 2001).
2.6. Examination of right ventricular hypertrophy
Right ventricular hypertrophy is a well-established index of PHT (Fulton and
Hutchinson, 1952), and has been shown to closely correlate with medial thickening of distal
pulmonary arteries in hypoxia-exposed rats (Rabinovitch et al., 1979; Rabinovitch et al., 1981).
At sacrifice, the thoracic contents were removed en bloc. The heart was then separated from the
lungs, the atria removed just inferior to the atrio-ventricular valves and discarded and the right
ventricle was dissected free from the left ventricle and septum. Each component was freeze-
33
dried and weighed separately and RVH was measured using the right ventricle/ (left ventricle +
septum) dry weight ratio as a marker (Kantores et al., 2006).
2.7. Percent medial wall thickness
Percentage arterial medial wall thickness (% MWT) was used as a marker of pulmonary
vascular remodelling (Ambalavanan et al., 2008; Xue et al., 2008; Mercier et al., 2009; Zhai et
al., 2009). Pulmonary arteries, identified by the presence of both inner and outer elastic lamina
using Hart’s elastin stain (detailed below). Images were digitally captured (Pixera Penguin
600CL, San Jose, CA) and analysis was undertaken by an observer blinded to group identity.
Vessel sizes of less than 20 µm or larger than 80 µm in external diameter were excluded, and at
least 20 vessels per animal were analysed. Mean external diameter was calculated from
measurements of round and ovoid vessels in two perpendicular planes (to account for any
irregularities in vessel shape), excluding vessels which were cut tangentially (more than three-
fold difference in MWT between perpendicular planes). Percent medial wall thickness was
measured using the formula: medial wall thickness x 2/mean external diameter x 100
(Rabinovitch et al., 1979).
2.8. Immunohistochemistry
Four randomly selected animals from each group were anaesthetised with intraperitoneal
(i.p.) ketamine (80 mg/kg) and xylazine (20 mg/kg) injections. After opening of the thoracic
cavity and cannulation of the trachea, the pulmonary veins were divided. The pulmonary
circulation was flushed with 1 × phosphate buffered saline (PBS) containing 1 U/ml heparin to
clear the lungs of blood, and perfusion fixed with 4% (w/v) neutral buffered paraformaldehyde
while inflated with air at a constant airway pressure of 20 cm H2O which was maintained via a
34
tracheal catheter. Paraffin-embedded tissues were cut into 5-µm sections and mounted on
Superfrost/Plus slides, allowed to air dry and baked overnight at 43°C. Sections were then
immersed in xylene (3 × 10 min) and rehydrated starting with 100% ethanol (3 × 5 min),
followed by 5 min each of 95, 90, 80, 70, and 50% ethanol. After washing (1 × PBS for 3 × 5
min), sections were boiled in 10 mM Na citrate for antigen retrieval. Slides were then immersed
for 30 min in 100% methanol with 0.3% (v/v) H2O2 to quench endogenous peroxidases. After
further washing, sections were blocked with 1% BSA (w/v)/5% NGS (v/v) for 1 h followed by
overnight incubation at 4°C with primary antibody or, where available, by pre-incubation with
the appropriate blocking peptide, according to the manufacturer’s instructions. Following
further washing, sections were incubated with biotin-conjugated secondary antisera diluted to
1:200 with blocking solution, at room temperature for 2 h. Sections were then washed and
incubated with avidin-biotin-peroxidase complex using the Vectastain ABC system, according
to the manufacturer’s instructions, at room temperature for 1-2 h. Finally, sections were stained
for 30 s to10 min with DAB. After further washing, sections were lightly counterstained with
Carazzi hematoxylin and rinsed in water for 15 min. Sections were dehydrated, cleared in
xylene and mounted using Permount. Images from stained sections were digitally captured
using a Zeiss Axioskop upright microscope (Carl Zeiss Inc., Oberkochen, Germany) equipped
with a Penguin 600CL camera and Viewfinder capture software (Pixera Corp., Los Gatos, CA).
2.9. Hart’s elastin staining
Paraffin-embedded tissue sections were de-waxed and rehydrated, followed by several
rinses with distilled water, and left overnight for 20 hours in Weigert’s resorcin-fuchsin stain
(Rowley Biochemical, Danvers, MA, U.S.A.). Slides were then washed in distilled water for 10
35
min, followed by counterstaining in tartrazine for 3 minutes. Slides were then dehydrated and
mounted by coverslip using a 50%/50% Permount/xylene solution. Images were digitally
captured as described above.
2.10. Western blot analyses
Whole (flash frozen) lung tissue or third-fourth generation PAs (dissected from 4 litters per
group; the pooled vessels of 2-3 animals from each litter representing 1 sample) were
homogenised and sonicated (40 W for 30 s) in RIPA cell lysis buffer (10 mM NaPO4, 0.3 M
NaCl, 0.1% (w/v) sodium dodecyl sulphate (SDS), 1% (v/v) Nonidet P-40, 1% (v/v) sodium
deoxycholate, 2 mM EDTA, pH 7.2) containing protease inhibitors (Protease Inhibitor Cocktail
Set I, EMD Chemicals, Gibbstown, NJ) and phosphatase inhibitor cocktail (Sigma). The
homogenate was left on ice for 10 min before centrifugation at 7,000 × g for 10 min. The
supernatant was then collected and protein concentration measured by a commercially-available
spectrophotometric assay using known concentrations of BSA as standards (Bradford, 1976).
Samples were then aliquoted and stored at -80°C until analysis. Tissue containing 50-100 µg of
protein was boiled for 5 min in SDS sample buffer (60 mM Tris-HCl, 10% (w/v) SDS, 5% (v/v)
glycerol, 2 mM β-mercaptoethanol, pH 6.8) and fractionated under reducing conditions by SDS
polyacrylamide gel electrophoresis for 2 h at 120 V. Following electrophoresis, proteins were
transferred to PVDF membranes. All membranes were blocked with 5% (v/v) Tween 20
overnight at 4°C and incubated with the appropriate primary antibodies for > 1 h at room
temperature. Blots were then washed in TBST and placed in secondary antibody for > 1 h at
room temperature.
36
Increased ROCK activity, characterised by an increased ratio of phosphorylated MLC-2:
unphosphorylated MLC-2, was assessed by using an acrylamide-pendant Phos-tagTM
ligand in
an SDS-PAGE system. This specialised variation on Western blot analysis incorporates a di-
nuclear metal complex, Mn2+
-Phos-tagTM
, into the gel matrix of a standard SDS-PAGE Western
blot. This allows for the elucidation of a ratio between phosphorylated to unphosphorylated
proteins of a particular sample on the same Western blot; in this case, the detection of
phosphorylated MLC-2 protein. A concentration of 5 mM of Mn2+
-Phos-tagTM
was incorporated
into a 12.5% acrylamide gel. Proteins were run under a constant current of 30mA, and then
transferred to PVDF membranes overnight at 4C under a constant voltage of 27 V. Following
electrophoresis and transfer, membranes were blotted with anti-MLC-2, yielding two bands (an
upper band representing phosphorylated and a lower band representing unphosphorylated MLC-
2). For each sample, density of the upper band was expressed as a ratio of the combined
densities of the upper and lower bands. After blotting, protein bands were imaged using an
enhanced chemiluminescence kit (Amersham Pharmacia Biotech, Piscataway, NJ, U.S.A.) and
exposed on Kodak X-OmatTM
Blue XB-1 film (Eastman Kodak, Rochester, NY, U.S.A.). Film
was electronically scanned and band density was quantified using Image J software (NIH,
Bethesda, MD, U.S.A.). Compensation for differences in protein loading was achieved by re-
blotting for GAPDH, and expressing results after normalisation to the GAPDH band.
2.11. Pulmonary artery smooth muscle cell (PASMC)-enriched culture
PASMCs were isolated using pulmonary artery explants from the pooled pulmonary
arteries of a litter (10-12 pups) of day 14 Sprague-Dawley rats, by a modification of a
previously described method (Jones & Rabinovitch, 1996). Pulmonary arteries were harvested,
37
opened with fine scissors, and the endothelium was scraped off by repeatedly rubbing the
luminal side with a scissor edge. The arteries were minced with scissors and washed in 1 × PBS
(pH 7.6) with antibiotic-antimycotic solution (10 U/ml penicillin G sodium, 10 µg/ml
streptomycin sulphate, 0.25 µg/ml amphotericin B, and 0.1 mg/ml gentamicin sulphate). Tissue
was placed in DMEM with 20% (v/v) FBS and antibiotic-antimycotic solution, and incubated
for 1-2 weeks at 37°C at a gas phase of 21% O2, 5% CO2, and 74% N2 until the cells had
attached. Cells were then passaged by trypsinisation using 0.05% (w/v) trypsin/EDTA and
centrifugation at 300 × g for 5 min, then reseeding. PASMCs were identified by their
characteristic hill-and-valley morphology and positive immunostaining for α-smooth muscle
actin. All experiments using PASMCs from the same litter were performed using cells from the
first passage. Equal numbers of cells (105 cells per well) were seeded in 96-well plates and
grown to semi-confluence with 10% (v/v) FBS and then serum-starved for 48 h. PASMCs were
incubated with DMEM alone (control) or DMEM with various concentrations of Y-27632, 10%
(v/v) FBS or Paclitaxel for 24 h. Values are means ± SEM for 6 wells per experiment. All
experiments were performed in duplicate, using cells derived from a different litter to ensure
reproducibility of results.
2.12. Terminal dUTP nick-end labelling (TUNEL) assay
PASMCs or frozen lung sections were examined for apoptotic cells using a
commercially-available TUNEL assay. For collection of frozen lung sections, two randomly
selected animals from each group were anaesthetised with i.p. ketamine (80 mg/kg) and
xylazine (20 mg/kg). After opening of the thoracic cavity and cannulation of the trachea, the
pulmonary veins were divided. The pulmonary circulation was flushed with 1 × PBS containing
38
1 U/ml heparin to clear the lungs of blood, as the lungs were inflated with frozen tissue matrix
(Tissue-Tek OCT®, Sakura Finetek, Torance, CA, U.S.A.), diluted 1:3 with 20% (w/v) sucrose
in PBS. The heart and lungs were then removed en bloc and covered with OCT® matrix using a
plastic mold placed on dry ice until the tissue and matrix were frozen, and stored at -80°C until
sectioning. Frozen lung tissue, cut by cryostat in to 15-20 µm-thick sections and placed on
SuperFrost/Plus slides or cultured PASMCs seeded on to Lab-Tek™ chamber slides (VWR,
Mississauga, ON, Canada) were stained with fluorescein, according to the manufacturer’s
instructions. Slides were then mounted with fluorescent mounting medium and digitally
photographed using an epifluorescent microscope (Zeiss Axioskop) with appropriate filter sets
(Fluorescein: excitation 495 nm and emission 520 nm; DAPI: excitation 350 nm and emission
470 nm).
2.13. Apoptosis-detection ELISA
Quantification of apoptosis in PASMCs was achieved using a commercially-available
ELISA designed to detect ssDNA (Cell Death Detection ELISAPLUS
, Roche). Cells were
seeded at a concentration of 2 105cells/ml, and incubated until sub-confluent, following which
they were trypsinised, washed and diluted with 20% FBS in DMEM culture medium to
neutralise trypsin. Y-27632 at concentrations of 0.1, 1, and 10 µM or a prototypic apoptosis-
inducer, Paclitaxel (10 µM; used as a positive control) in DMEM were added to the PASMCs,
and incubated at 37°C for 24 h. Following incubation, microplates were centrifuged, the cell
pellet combined with lysis buffer, and incubated at room temperature for 30 minutes. The lysate
was then centrifuged for 10 minutes, and the supernatant transferred on to a streptavidin-coated
microplate. Immunoreagent was added to each well, followed by incubation at room
39
temperature with gentle shaking. The wells were then emptied and washed with incubation
buffer, and 2, 2´-azino-bis-(3-benzthiazoline-6-sulfonic acid) (ABTS) solution was added. The
microplate was then incubated at room temperature with gentle shaking for 10-20 minutes, or
until colour development, followed by the addition of the ABTS Stop solution. Optical density
was measured by plate reader at a wavelength of 405 nm.
2.14. Cell viability assay
PASMC proliferation was quantified using the Wst-8 cell proliferation assay kit
(Cayman Chemicals). Cells were seeded in a 96-well plate at a concentration of 105 cells per
well, and treated with DMEM alone, DMEM with 20% (v/v) FBS, or DMEM with Y-27632 at
concentrations of 0.1, 1, and 10 µM. for 24 h. Reconstituted Wst-8 mixture was added to each
well, and the plate was put on a shaker at low speed for 1 minute, followed by an incubation
period of 2 hours at 37°C. Optical density was measured in a spectrophotometer using a
wavelength of 405 nm.
2.15. Data presentation and analysis
All values are expressed as the mean ± standard error of the mean (SEM). For in vitro
studies of cultured PASMCs, at least one replicate experiment using pooled explants from a
different litter of pups was performed to demonstrate reproducibility of results. Statistical
significance (p< 0.05) was determined using Sigma Stat 3.0 software (SPSS, Chicago, IL,
U.S.A.) using one-way analysis of variance (ANOVA) followed by pair-wise multiple
comparisons using the Tukey’s test when significant differences were found (Snedecor, 1968;
Glantz, 2002).
41
3.1. Body weight
Hypoxia-exposed animals, regardless of whether they received vehicle or Y-27632, had
significantly lower body weights when compared to air-exposed animals. Treatment with Y-
27632 had no impact on body weight in either group (Fig. 14).
3.2. Pulmonary vascular resistance
Hypoxia-exposed, vehicle-treated animals had significantly higher PVR values when
compared to air-exposed, vehicle-treated animals (Fig. 15). PVR was completely normalized in
animals exposed to hypoxia and treated with Y-27632. Animals exposed to air and treated with
Y-27632 had similar PVR values compared to vehicle-treated controls.
3.3. Pulmonary artery systolic pressure
Hypoxia-exposed, vehicle-treated animals had significantly higher PASP compared to
air-exposed, vehicle-treated animals (Fig. 16). Animals treated with Y-27632 and exposed to
hypoxia had significantly lower PASP compared to vehicle-treated animals. Animals exposed
to air and treated with Y-27632 had similar PASPs compared to vehicle-treated controls.
42
Figure 14. Body weights. Body weights of day-21 rat pups. *p<0.001, by ANOVA, compared
to respective air-exposed groups, n=12 animals; representing 2 litters/group.
43
Figure 15. Pulmonary vascular resistance. Doppler-derived inverse ratio of pulmonary artery
acceleration time (PAAT) and right ventricular ejection time (RVET) as a measure of PVR in
day-21 rat pups. *p<0.001, by ANOVA, compared to all other groups. n=7-8 animals
representing 2 litters/group.
44
Figure 16. Pulmonary artery systolic pressure (PASP). PASP was estimated in day-21 rat
pups.*p<0.05, by ANOVA, compared to all other groups. #p<0.05, by ANOVA, compared to
air-exposed Y-27632-treated group. n=7-8 animals representing 2 litters/group.
45
3.4. Right ventricular performance
Hypoxia-exposed, vehicle-treated animals had significantly lower RVIs compared to air-
exposed, vehicle-treated animals (Fig. 17). Animals treated with Y-27632 and exposed to
hypoxia had values comparable to air-exposed controls. Animals exposed to air and treated
with Y-27632 had RVIs comparable to air-exposed, vehicle-treated controls.
3.5. Right ventricular hypertrophy
Hypoxia-exposed, vehicle-treated animals developed significant RVH when compared to
air-exposed, vehicle-treated animals (Fig. 18). Animals treated with Y-27632 and exposed to
hypoxia had significantly attenuated RVH compared to vehicle-treated hypoxia-exposed
animals.
3.6. Arterial wall remodelling
Hypoxia-exposed, vehicle-treated animals had significantly higher %MWT values than
air-exposed, vehicle-treated animals (Fig. 19). Hypoxia-exposed animals treated with Y-27632
had completely normalised %MWT values. Animals exposed to air and treated with Y-27632
had significantly decreased %MWT values when compared to air-exposed vehicle-treated
animals. Representative Hart’s elastin stained sections are shown in Figure 20.
46
Figure 17. Right ventricular performance index. Right ventricular index, as a measure of right
ventricular output, in day-21 rat pups. *p<0.05, by ANOVA, compared to other groups, n=7-8
animals representing 2 litters/group.
47
Figure 18. Right ventricular hypertrophy (RVH). Right ventricle (RV)/left ventricle + septum
(LV+S) weight ratio as a marker of RVH in day-21 rat pups. *p<0.001, by ANOVA, compared
to all other groups, #p<0.01, by ANOVA, compared to air-exposed groups, n=7 animals
representing 2 litters/group.
48
Figure 19. Percent medial wall thickness (% MWT). % MWT was derived from day-21 lung
sections stained with Hart’s elastin stain. *p<0.001, by ANOVA, compared to all other groups,
and #p<0.05, by ANOVA, compared to air-exposed vehicle-treated group, n=4 animals
representing 2 litters/group.
49
Figure 20. Hart’s elastin stain. Hart’s elastin staining for elastin (dark brown) and tartrazine
counterstain (light brown) in paraffin-embedded lung tissue from day-21 rat pups.
50
3.7. Prepro-ET-1 immunohistochemistry
Animals exposed to hypoxia and treated with vehicle had increased vascular wall prepro-
ET-1 immunoreactivity compared to animals exposed to air and treated with vehicle (Fig. 21).
Animals treated with Y-27632, whether exposed to hypoxia or air, had comparable prepro-ET-1
immunoreactivity to air-exposed, vehicle-treated animals.
3.8. Prepro-ET-1 content
Consistent with findings on immunohistochemistry, Western blot analyses of pulmonary
arterial prepro-ET-1 showed increased prepro-ET-1 content in hypoxia-exposed vehicle-treated
animals when compared to air-exposed groups and hypoxia-exposed animals treated with Y-
27632 (Fig. 22).
3.9. ROCK-I and ROCK-II content
No changes in pulmonary arterial ROCK-I (Fig. 23) or ROCK-II (Fig. 24) content were
observed between groups.
3.10. MLC-2 phosphorylation
Hypoxia-exposed, vehicle-treated animals had significantly increased MLC-2
phosphorylation, as a marker of ROCK activity, compared to air-exposed, vehicle-treated
animals (Fig. 25). In hypoxia-exposed animals treated with Y-27632, MLC-2 phosphorylation
was completely normalised, indicating that Y-27632 completely attenuated the hypoxia-
mediated increase in ROCK activity. Animals exposed to air and treated with Y-27632 had no
change in MLC-2 phosphorylation compared to air-exposed controls.
51
Figure 21. Prepro-ET-1 immunostaining. Immunohistochemical staining for the ET-1
precursor, prepro-ET-1 (dark brown) and hemotoxylin (light blue) in paraffin-embedded lung
tissue of postnatal day-21 control and Y-27632-treated rat pups. Inset image. Hypoxia vehicle-
treated negative control.
52
Figure 22. Prepro-ET-1 content. Top. Prepro-ET-I content in pulmonary arterial tissue of
postnatal day-21 control and Y-27632-treated rat pups. Bottom. Representative Western blots.
Molecular weight of Prepro-ET-1 is 24.4 kDa. *p<0.01, by ANOVA, compared to all other
groups, n=4 samples/group.
53
Figure 23. ROCK-I content. Top. ROCK-I content in pulmonary arterial tissue of postnatal
day-21 control and Y-27632-treated rat pups. Bottom. Representative Western blots. Molecular
weight of ROCK-I is 160 kDa. n=4 samples/group.
54
Figure 24. ROCK-II content. Top. ROCK-II content in pulmonary arterial tissue of postnatal
day-21 control and Y-27632-treated rat pups. Bottom. Representative Western blots. Molecular
weight of ROCK-II is 160 kDa. n=4 samples/group.
55
Figure 25. Rho-kinase activity. Top. MLC-2 phosphorylation in pulmonary arterial tissue of
postnatal day-17 control and Y-27632-treated rat pups, as a marker of Rho-kinase activity.
Bottom. Representative immunoblots for MLC-2 using Phos-tag Western blot analysis.
*p<0.001, by ANOVA, compared to all other groups, n=4 samples/group.
56
3.11. PASMC proliferation
Compared to control (DMEM only)-treated PASMCs, cells treated with Y-27632 (1 and
10 µM) had significantly decreased proliferation when compared to positive controls (Fig. 26).
3.12. Ki-67 immunohistochemistry
Ki-67 immunostaining was used to identify cells undergoing DNA synthesis. Increased
numbers of proliferating medial arterial wall smooth muscle cells were observed in vessels of
animals exposed to hypoxia and treated with vehicle when compared to all other groups (Fig.
27).
3.13. In vitro TUNEL assay and ELISA for apoptosis
Treatment with Y-27632 led to greatly increased apoptosis in PASMCs when compared
to untreated controls (Fig. 28). This finding was confirmed using quantitative ELISA (Fig. 29).
3.14. In vivo TUNEL assay
Using fluorescent TUNEL on day-17 frozen lung tissue to identify cells undergoing
apoptosis increased apoptosis was observed in the arterial walls of both air- and hypoxia-
exposed animals treated with Y-27632 when compared to vehicle-treated animals (Fig. 30).
57
Figure 26. Proliferation index. Proliferation index of primary cultures of PASMCs using a
colorimetric assay. *p<0.05, by ANOVA, compared to Y-27632-free negative control group.
The positive controls were cells placed in 10% FBS for 24 hours.
58
Figure 27. Immunohistochemical staining for Ki67, a marker for DNA synthesis. Ki67-positive
staining (dark brown) and hemotoxylin (light blue) in paraffin-embedded lung tissue from
postnatal day-17 control and Y-27632-treated rat pups. Black arrows point to two Ki67-positive
cells in the medial arterial wall.
59
Figure 28. Apoptosis in primary cultures of PASMC. Fluorescent TUNEL stain showing
increased apoptotic nuclei (green) in primary cultured PASMCs treated with Y-27632. Positive
control cells were treated with DNAse I.
60
Figure 29. Apoptosis index. Apoptosis index of primary cultures of PASMCs measured by
colorimetric ELISA. *p<0.001 compared to all other groups, #p<0.001 compared to negative
control group. Positive control cells were treated with 10 µM Paclitaxel.
61
Figure 30. Apoptosis marker in frozen tissue sections. Fluorescent TUNEL assay to identify
apoptotic nuclei (green). Non-apoptotic nuclei are stained by DAPI (blue) in postnatal day-17
frozen lung tissue of control and Y-27632-treated air-exposed and hypoxia-exposed rat pups;
pa= pulmonary artery.
63
The aims of this project were to examine whether sustained treatment with a ROCK inhibitor,
Y-27632, would normalise PVR, augment RV performance, and reverse vascular remodelling in
a neonatal chronic hypoxic rat model of PHT. As hypothesised, treatment with Y-27632
reversed the structural (RVH and arterial wall remodelling, as reflected by %MWT) and
functional (raised PVR and attenuated RV performance) abnormalities of chronic hypoxic PHT.
Our finding that Y-27632 led to quantitatively increased apoptosis and decreased proliferation
of PASMCs in vitro and qualitative differences in vivo provides a mechanistic explanation for
the reversal of established structural changes of vascular remodelling. Therefore, our results
point towards a structural as well as a functional attenuation of chronic hypoxic PHT, which
may be due to the effectiveness of Y-27632 both as a vasodilator and as a pro-apoptotic/anti-
proliferative agent. Moreover, normalisation of RV performance with Y-27632 has not, to our
knowledge, been observed in any previous studies examining treatments for established chronic
PHT in adult animals, including other ROCK inhibitors, such as Fasudil. Together, our findings
could have important therapeutic implications for chronic forms of PHT in infancy and
childhood, because severe vascular remodelling is a pathological hallmark of fatal PHT and RV
dysfunction carries a high risk of early death (Utsunomiya et al., 2009).
The observed vasodilatory effects of Y-27632 are likely to be caused by the inhibition of
the RhoA/ROCK-mediated pathway (Fig. 3) Ca2+
sensitisation by Y-27632, in which MLC-2
becomes phosphorylated (Hanazaki et al., 2008). If ROCK is activated, as it is in this chronic
hypoxic model, the inhibition of this pathway would thereby lead to the attenuation of sustained
vasoconstriction. Other possible contributing factors, not tested in this thesis, include attenuated
actin polymerization and/or augmented function of the NO-cGMP pathway. ROCK inhibition
may also contribute to a decrease in the number of vascular SMCs, as ROCK is involved in
64
many cellular processes, including mitogenesis (Liu et al., 2004). A decrease in the number of
vascular SMCs, or a cessation of the proliferation of such cells, would thus lead to an
attenuation of vascular remodelling. Previous research examining production of endothelin-1 by
pulmonary artery SMCs in response to thromboxane (TXA2) receptor stimulation with 8-
isoprostane, has demonstrated that treatment with Y-27632 resulted in a decrease in ET-1
production and release (Yi et al., 2006). Interestingly, the same tissues exhibiting increased ET-
1 expression also exhibited increased ROCK activity, which was attenuated through treatment
with the ROCK inhibitor Y-27632. The importance of this finding is the overwhelming
evidence that ET-1 plays an important role in PHT development both in newborn and adult
experimental models (Jankov et al., 2000; Porchia et al., 2008), such that ET-1 receptor
antagonists are now an established therapy for children and adults with chronic PHT (Rubin et
al., 2002; Barst et al., 2006). Thus, a relationship between ROCK and ET-1 could potentially
explain the effects of ROCK inhibition on promoting apoptosis of SMCs, as it is known that
along with having a vasoconstrictive role, ET-1 also promotes SMC growth and survival
through the inhibition of apoptosis (Wu-Wong et al., 1997; Jankov et al., 2000; Jankov et al.,
2006). Therefore, treatment with Y-27632 may induce apoptosis, at least in part, by attenuating
ET-1 expression. Other mechanisms for putative actions of ROCK as an anti-apoptotic
molecule have also been postulated, particularly in the fields of cancer and tumorigenesis.
Effects on the expression of p53 protein (Xue et al., 2007), the activation and release of
caspases through mitochondrial membrane depolarisation (Maeda et al., 2009), as well as the
inhibition of the proper adhesion of cells for continued growth (Rattan et al., 2006) have all
been proposed as possible mechanisms for the pro-apoptotic effects of Y-27632 that could also
apply to SMC apoptosis.
65
Concerning the mechanisms of Y-27632-induced attenuation of chronic hypoxia-induced
RV dysfunction, it could be inferred that a decrease in RV afterload helped significantly in
improving RV function, although other mechanisms may have contributed. It has been shown
by Sugiyama and colleagues (Sugiyama et al., 2002) that Y-27632 enhances heart function by
improving sinoatrial automaticity, increasing coronary blood flow and reducing myocardial O2
demand through altered myofibrillar Ca2+
sensitivity. Y-27632 has also been reported to
attenuate increased myocardial contractility (and thus O2 demand) caused by the administration
of ET-1, angiotensin-II, or prostaglandin F2α, all of which are powerful vasoconstrictors
(Nishimaru et al., 2003). This attenuation was believed to result from two mechanisms: the
inhibition of α-adrenoceptor-mediated increased Ca2+
sensitivity, and/or from the decrease of a
Na2+
/H+ exchanger that was found to be activated together with the RhoA/ROCK pathway
(Nishimaru et al., 2003). Therefore, it is possible that Y-27632 exerted direct effects on the
myocardium in addition to reducing afterload through attenuation of Ca2+
sensitisation.
In previous work, our laboratory has studied the acute haemodynamic effects of a single
bolus of Y-27632 on hypoxia- and bleomycin-induced chronic neonatal PHT models
(McNamara et al., 2008). Y-27632 resulted in completely normalised PVR but did not improve
RV output/function. Subsequently, the effects of Y-27632 when given from birth at the onset of
chronic hypoxic exposure were examined (Ziino et al., 2010). The results of this study showed
that there was also attenuation of PVR, RVH, and vascular remodelling (at least in part through
inhibitory effects of PDGF-β receptor signaling), indicating that ROCK is a critical initiating
factor in the pathogenesis of hypoxia-induced vascular remodelling. In addition, no adverse
effects on lung growth and development were observed in Y-27632-treated animals during a
period when the increase in alveolar density is maximal in the rat (Ziino et al., 2010). The study
66
outlined in this thesis represented a logical continuum of previous work, whereby the reversing
effects of Y-27632 were examined once chronic hypoxic PHT was already well-established.
Collectively, these studies strongly suggest that Y-27632, and possibly other inhibitors of
ROCK, have potential as a novel treatment for PHT in infancy and childhood that is non-
responsive to conventional therapies.
4.1. Limitations and future research
Much remains to be understood about the involvement of ROCK in chronic PHT in
human infants and children and the possible side-effects of ROCK inhibitors, prior to clinical
translation. For example, systemic administration of ROCK inhibitors from birth was found to
worsen somatic growth restriction in chronic hypoxia-exposed pups (Ziino et al., 2010), which
has not been reported in mature rodents receiving either Y-27632 or Fasudil. Evidence from
that study strongly suggested that growth restriction was related to systemic inhibition of
ROCK, rather than through an off-target effect of Y-27632 (Ziino et al., 2010). We believe that
systemic hypoperfusion, due to parallel dilating effects of ROCK inhibitors on the systemic
vasculature (Nagaoka et al., 2005), is likely to account for many adverse effects, including
growth restriction. Importantly, in the present study, treatment with Y-27632 caused no adverse
effects on somatic growth, which is likely explained by the different timing of treatments (days
14-21, rather than days 1-14 of life). In pilot dose-response studies carried out at 14 days of life,
we observed immediate ill effects consistent with hypotensive shock, including gray pallor,
weakness, decreased activity and (in many cases) death. These effects were more frequent and
severe the higher the dose (30 mg/kg>>25 mg/kg>>20 mg/kg), appeared to be worse in air-
exposed animals than in animals chronically exposed to hypoxia, and were not observed at 15
67
mg/kg, which was the dose ultimately used in the present study. We chose to perform twice
daily injections of Y-27632, given that studies in adult rodents suggest inhibitory effects on
ROCK activity (as measured by vasodilatory effects on the pulmonary circulation) last
approximately 4-6 hours after a single bolus injection (Nagaoka et al., 2004).
ROCK is known to be expressed in both vascular and non-vascular cell types in many
tissues; therefore, it is likely that ROCK mediates many processes in cell types other than
vascular SMCs, including cell motility, adhesion and proliferation. Therefore, the need for
more information concerning systemic effects of ROCK inhibition is evident. Furthermore,
given the apparent increased sensitivity of newborn animals to the systemic effects of ROCK
inhibitors and the narrow therapeutic-toxic dose range, our results suggest that systemic
treatment with this class of agents should be undertaken in neonates and infants with caution. A
potentially safer and equally efficacious approach may be through delivery of smaller doses
directly to the lung, either by intratracheal instillation (similar to exogenous surfactant) or by
nebulisation, which has been shown in adult animals to limit associated effects on the systemic
vasculature (Nagaoka et al., 2005).
Chronic PHT is a complex disease with multiple factors contributing to pathogenesis,
including hypoxia, inflammation, and the underdevelopment of the pulmonary vasculature.
Therefore, it would be important to confirm the present findings in models of neonatal PHT in
which inflammation is critical, including chronic exposure to hyperoxia or systemic treatment
with bleomycin (Yi et al., 2004; McNamara et al., 2008; Tourneux et al., 2008). Additionally,
longer-term studies are required to determine whether the beneficial effects of Y-27632 last
beyond the treatment period and whether combining Y-27632 with existing treatments, such as
iNO, would enhance its effects.
68
A complete understanding of the role in the RhoA/ROCK pathway in the initiation and
persistence of chronic PHT is lacking; therefore, examination of the effects of more possible
upstream and/or downstream effector molecules of ROCK is needed to pinpoint how and where
ROCK contributes to the pathogenesis of PHT. Some of these molecules include: GEF, GDI,
GAP, MAPK, LIMK, cofilin, CPI-17, and many other proteins and enzymes that were discussed
earlier. The examination of the role of ROCK can also be more precisely elucidated through the
use of siRNA-mediated knockdown or conditional knockout animal models. Currently, there
exist both ROCK-I and ROCK-II knockout mice. ROCK-I knockouts exhibit defects in eyelid
epithelia while the loss of ROCK-II expression results in placental dysfunction, leading to
intrauterine growth restriction (Thumkeo et al., 2005). Interestingly, in contrast to the effect of
ROCK inhibition in the lung, it was observed that in mouse models of systemic hypertension,
deletion of ROCK-I expression resulted in reduced cardiac fibrosis, and reduced cardiomyocyte
apoptosis, even though an increase of apoptosis was observed in the lung in hypertensive
models (Chang et al., 2006), suggesting differing effects of ROCK in various organ systems.
Thus, it would be useful in the future to use conditional knockouts or siRNA-induced models for
the study of PHT development, which might allow for the specific knockdown of ROCK in the
lungs only.
Though much remains to be understood before ROCK inhibitors may be introduced into
clinical practice, this project yielded many promising and important results that may drive future
research aimed at increasing our understanding about the effects of ROCK inhibitors in the
neonate. With an improved understanding of the optimal dose, mode of administration and
associated effects, ROCK inhibitors could have great potential as a testable therapy in patients
who are non-responsive to current treatments for chronic PHT.
69
REFERENCE LIST
Abe K, Shimokawa H, Morikawa K, Uwatoku T, Oi K, Matsumoto Y, Hattori T, Nakashima Y,
Kaibuchi K, Sueishi K & Takeshit A (2004). Long-term treatment with a Rho-kinase inhibitor
improves monocrotaline-induced fatal pulmonary hypertension in rats. Circ Res 94, 385-393.
Abe K, Tawara S, Oi K, Hizume T, Uwatoku T, Fukumoto Y, Kaibuchi K & Shimokawa H (2006).
Long-term inhibition of Rho-kinase ameliorates hypoxia-induced pulmonary hypertension in
mice. J Cardiovasc Pharmacol 48, 280-285.
Abman SH (2007). Recent advances in the pathogenesis and treatment of persistent pulmonary
hypertension of the newborn. Neonatology 91, 283-290.
Alano MA, Ngougmna E, Ostrea EM, Jr. & Konduri GG (2001). Analysis of nonsteroidal
antiinflammatory drugs in meconium and its relation to persistent pulmonary hypertension of the
newborn. Pediatrics 107, 519-523.
Ambalavanan N, Nicola T, Hagood J, Bulger A, Serra R, Murphy-Ullrich J, Oparil S & Chen YF (2008).
Transforming growth factor-beta signaling mediates hypoxia-induced pulmonary arterial
remodeling and inhibition of alveolar development in newborn mouse lung. Am J Physiol Lung
Cell Mol Physiol 295, L86-95.
Ananthakrishnan M, Barr FE, Summar ML, Smith HA, Kaplowitz MR, Cunningham G, Magarik J,
Zhang Y & Fike CD (2009). L-citrulline Ameliorates Chronic Hypoxia-induced Pulmonary
Hypertension in Newborn Piglets. Am J Physiol Lung Cell Mol Physiol.
Andersen A, Nielsen JM, Peters CD, Schou UK, Sloth E & Nielsen-Kudsk JE (2008). Effects of
phosphodiesterase-5 inhibition by sildenafil in the pressure overloaded right heart. Eur J Heart
Fail 10, 1158-1165.
Badesch DB, Abman SH, Ahearn GS, Barst RJ, McCrory DC, Simonneau G & McLaughlin VV (2004).
Medical therapy for pulmonary arterial hypertension: ACCP evidence-based clinical practice
guidelines. Chest 126, 35S-62S.
Balasubramaniam V, Le Cras TD, Ivy DD, Grover TR, Kinsella JP & Abman SH (2003). Role of
platelet-derived growth factor in vascular remodeling during pulmonary hypertension in the
ovine fetus. Am J Physiol Lung Cell Mol Physiol 284, L826-833.
Barst RJ, Langleben D, Badesch D, Frost A, Lawrence EC, Shapiro S, Naeije R & Galie N (2006).
Treatment of pulmonary arterial hypertension with the selective endothelin-A receptor antagonist
sitaxsentan. J Am Coll Cardiol 47, 2049-2056.
Belik J (2008). Fetal and neonatal effects of maternal drug treatment for depression. Semin Perinatol 32,
350-354.
Belik J, Jankov RP, Pan J & Tanswell AK (2004). Peroxynitrite inhibits relaxation and induces
pulmonary artery muscle contraction in the newborn rat. Free Radic Biol Med 37, 1384-1392.
70
Bogaard HJ, Abe K, Vonk Noordegraaf A & Voelkel NF (2009). The right ventricle under pressure:
cellular and molecular mechanisms of right-heart failure in pulmonary hypertension. Chest 135,
794-804.
Bradford MM (1976). A rapid and sensitive method for the quantitation of microgram quantities of
protein utilizing the principle of protein-dye binding. Anal Biochem 72, 248-254.
Broughton BR, Walker BR & Resta TC (2008). Chronic hypoxia induces Rho kinase-dependent
myogenic tone in small pulmonary arteries. Am J Physiol Lung Cell Mol Physiol 294, L797-806.
Burri PH (1974). The postnatal growth of the rat lung. 3. Morphology. Anat Rec 180, 77-98.
Caslin A, Heath D & Smith P (1991). Influence of hypobaric hypoxia in infancy on the subsequent
development of vasoconstrictive pulmonary vascular disease in the Wistar albino rat. J Pathol
163, 133-141.
Chambers CD, Hernandez-Diaz S, Van Marter LJ, Werler MM, Louik C, Jones KL & Mitchell AA
(2006). Selective serotonin-reuptake inhibitors and risk of persistent pulmonary hypertension of
the newborn. N Engl J Med 354, 579-587.
Chang J, Xie M, Shah VR, Schneider MD, Entman ML, Wei L & Schwartz RJ (2006). Activation of
Rho-associated coiled-coil protein kinase 1 (ROCK-1) by caspase-3 cleavage plays an essential
role in cardiac myocyte apoptosis. Proc Natl Acad Sci U S A 103, 14495-14500.
Chen XY, Dun JN, Miao QF & Zhang YJ (2009). Fasudil hydrochloride hydrate, a Rho-kinase inhibitor,
suppresses 5-hydroxytryptamine-induced pulmonary artery smooth muscle cell proliferation via
JNK and ERK1/2 pathway. Pharmacology 83, 67-79.
Chen YF, Feng JA, Li P, Xing D, Zhang Y, Serra R, Ambalavanan N, Majid-Hassan E & Oparil S
(2006). Dominant negative mutation of the TGF-beta receptor blocks hypoxia-induced
pulmonary vascular remodeling. J Appl Physiol 100, 564-571.
Chhina MK, Nargues W, Grant GM & Nathan SD (2010). Evaluation of imatinib mesylate in the
treatment of pulmonary arterial hypertension. Future Cardiol 6, 19-35.
Clark RH, Huckaby JL, Kueser TJ, Walker MW, Southgate WM, Perez JA, Roy BJ & Keszler M (2003).
Low-dose nitric oxide therapy for persistent pulmonary hypertension: 1-year follow-up. J
Perinatol 23, 300-303.
Clark RH, Kueser TJ, Walker MW, Southgate WM, Huckaby JL, Perez JA, Roy BJ, Keszler M &
Kinsella JP (2000). Low-dose nitric oxide therapy for persistent pulmonary hypertension of the
newborn. Clinical Inhaled Nitric Oxide Research Group. N Engl J Med 342, 469-474.
Corte TJ, Wort SJ, Gatzoulis MA, Macdonald P, Hansell DM & Wells AU (2009). Pulmonary Vascular
Resistance Predicts Early Mortality in Patients with Diffuse Fibrotic Lung Disease and
Suspected Pulmonary Hypertension. Thorax.
Curtis J, Kim G, Wehr NB & Levine RL (2003). Group B streptococcal phospholipid causes pulmonary
hypertension. Proc Natl Acad Sci U S A 100, 5087-5090.
71
Dakshinamurti S (2005). Pathophysiologic mechanisms of persistent pulmonary hypertension of the
newborn. Pediatr Pulmonol 39, 492-503.
Dalla-Favera R, Gallo RC, Giallongo A & Croce CM (1982). Chromosomal localization of the human
homolog (c-sis) of the simian sarcoma virus onc gene. Science 218, 686-688.
Davies SP, Reddy H, Caivano M & Cohen P (2000). Specificity and mechanism of action of some
commonly used protein kinase inhibitors. Biochem J 351, 95-105.
Do e Z, Fukumoto Y, Takaki A, Tawara S, Ohashi J, Nakano M, Tada T, Saji K, Sugimura K, Fujita H,
Hoshikawa Y, Nawata J, Kondo T & Shimokawa H (2009). Evidence for Rho-kinase activation
in patients with pulmonary arterial hypertension. Circ J 73, 1731-1739.
Doggrell SA (2005). Rho-kinase inhibitors show promise in pulmonary hypertension. Expert Opin
Investig Drugs 14, 1157-1159.
Eriksen V, Nielsen LH, Klokker M & Greisen G (2009). Follow-up of 5- to 11-year-old children treated
for persistent pulmonary hypertension of the newborn. Acta Paediatr 98, 304-309.
Evans NJ & Archer LN (1991). Doppler assessment of pulmonary artery pressure and extrapulmonary
shunting in the acute phase of hyaline membrane disease. Arch Dis Child 66, 6-11.
Fabris VE, Pato MD & Belik J (2001). Progressive lung and cardiac changes associated with pulmonary
hypertension in the fetal rat. Pediatr Pulmonol 31, 344-353.
Fagan KA, Oka M, Bauer NR, Gebb SA, Ivy DD, Morris KG & McMurtry IF (2004). Attenuation of
acute hypoxic pulmonary vasoconstriction and hypoxic pulmonary hypertension in mice by
inhibition of Rho-kinase. Am J Physiol Lung Cell Mol Physiol 287, L656-664.
Fakioglu H, Totapally BR, Torbati D, Raszynski A, Sussmane JB & Wolfsdorf J (2005). Hypoxic
respiratory failure in term newborns: clinical indicators for inhaled nitric oxide and
extracorporeal membrane oxygenation therapy. J Crit Care 20, 288-293.
Galaria, II, Fegley AJ, Nicholl SM, Roztocil E & Davies MG (2004). Differential regulation of ERK1/2
and p38(MAPK) by components of the Rho signaling pathway during sphingosine-1-phosphate-
induced smooth muscle cell migration. J Surg Res 122, 173-179.
Galie N, Ghofrani HA, Torbicki A, Barst RJ, Rubin LJ, Badesch D, Fleming T, Parpia T, Burgess G,
Branzi A, Grimminger F, Kurzyna M & Simonneau G (2005). Sildenafil citrate therapy for
pulmonary arterial hypertension. N Engl J Med 353, 2148-2157.
Glantz JC (2002). Clearing up meconium: clinical management and research ethics. Birth 29, 137-140.
Group TF-BCNT (1999). Early compared with delayed inhaled nitric oxide in moderately hypoxaemic
neonates with respiratory failure: a randomised controlled trial. The Franco-Belgium
Collaborative NO Trial Group. Lancet 354, 1066-1071.
Guilluy C, Eddahibi S, Agard C, Guignabert C, Izikki M, Tu L, Savale L, Humbert M, Fadel E, Adnot S,
Loirand G & Pacaud P (2009). RhoA and Rho kinase activation in human pulmonary
hypertension: role of 5-HT signaling. Am J Respir Crit Care Med 179, 1151-1158.
72
Hampl V & Herget J (1990). Perinatal hypoxia increases hypoxic pulmonary vasoconstriction in adult
rats recovering from chronic exposure to hypoxia. Am Rev Respir Dis 142, 619-624.
Hanazaki M, Chiba Y, Yokoyama M, Morita K, Kohjitani A, Sakai H & Misawa M (2008). Y-27632
augments the isoflurane-induced relaxation of bronchial smooth muscle in rats. J Smooth Muscle
Res 44, 189-193.
Haniu M, Hsieh P, Rohde MF & Kenney WC (1994). Characterization of disulfide linkages in platelet-
derived growth factor AA. Arch Biochem Biophys 310, 433-437.
Haniu M, Rohde MF & Kenney WC (1993). Disulfide bonds in recombinant human platelet-derived
growth factor BB dimer: characterization of intermolecular and intramolecular disulfide
linkages. Biochemistry 32, 2431-2437.
Haworth SG (1988). Pulmonary vascular remodeling in neonatal pulmonary hypertension. State of the
art. Chest 93, 133S-138S.
Hoeper MM, Tongers J, Leppert A, Baus S, Maier R & Lotz J (2001). Evaluation of right ventricular
performance with a right ventricular ejection fraction thermodilution catheter and MRI in
patients with pulmonary hypertension. Chest 120, 502-507.
Humbert M, Monti G, Fartoukh M, Magnan A, Brenot F, Rain B, Capron F, Galanaud P, Duroux P,
Simonneau G & Emilie D (1998). Platelet-derived growth factor expression in primary
pulmonary hypertension: comparison of HIV seropositive and HIV seronegative patients. Eur
Respir J 11, 554-559.
Hyvelin JM, Howell K, Nichol A, Costello CM, Preston RJ & McLoughlin P (2005). Inhibition of Rho-
kinase attenuates hypoxia-induced angiogenesis in the pulmonary circulation. Circ Res 97, 185-
191.
Ishikura K, Yamada N, Ito M, Ota S, Nakamura M, Isaka N & Nakano T (2006). Beneficial acute effects
of rho-kinase inhibitor in patients with pulmonary arterial hypertension. Circ J 70, 174-178.
Ishizaki T, Uehata M, Tamechika I, Keel J, Nonomura K, Maekawa M & Narumiya S (2000).
Pharmacological properties of Y-27632, a specific inhibitor of Rho-associated kinases. Mol
Pharmacol 57, 976-983.
Jaffe AB & Hall A (2005). Rho GTPases: biochemistry and biology. Annu Rev Cell Dev Biol 21, 247-
269.
Jankov RP, Kantores C, Belcastro R, Yi M & Tanswell AK (2006). Endothelin-1 inhibits apoptosis of
pulmonary arterial smooth muscle in the neonatal rat. Pediatr Res 60, 245-251.
Jankov RP, Luo X, Cabacungan J, Belcastro R, Frndova H, Lye SJ & Tanswell AK (2000). Endothelin-1
and O2-mediated pulmonary hypertension in neonatal rats: a role for products of lipid
peroxidation. Pediatr Res 48, 289-298.
Jones JE, Mendes L, Rudd MA, Russo G, Loscalzo J & Zhang YY (2002). Serial noninvasive
assessment of progressive pulmonary hypertension in a rat model. Am J Physiol Heart Circ
Physiol 283, H364-371.
73
Jones PL & Rabinovitch M (1996). Tenascin-C is induced with progressive pulmonary vascular disease
in rats and is functionally related to increased smooth muscle cell proliferation. Circ Res 79,
1131-1142.
Kantores C, McNamara PJ, Teixeira L, Engelberts D, Murthy P, Kavanagh BP & Jankov RP (2006).
Therapeutic hypercapnia prevents chronic hypoxia-induced pulmonary hypertension in the
newborn rat. Am J Physiol Lung Cell Mol Physiol 291, L912-922.
Keith IM, Tjen ALS, Kraiczi H & Ekman R (2000). Three-week neonatal hypoxia reduces blood CGRP
and causes persistent pulmonary hypertension in rats. Am J Physiol Heart Circ Physiol 279,
H1571-1578.
Khemani E, McElhinney DB, Rhein L, Andrade O, Lacro RV, Thomas KC & Mullen MP (2007).
Pulmonary artery hypertension in formerly premature infants with bronchopulmonary dysplasia:
clinical features and outcomes in the surfactant era. Pediatrics 120, 1260-1269.
King AP, Smith P & Heath D (1995). Ultrastructure of rat pulmonary arterioles after neonatal exposure
to hypoxia and subsequent relief and treatment with monocrotaline. J Pathol 177, 71-81.
Kourembanas S, McQuillan LP, Leung GK & Faller DV (1993). Nitric oxide regulates the expression of
vasoconstrictors and growth factors by vascular endothelium under both normoxia and hypoxia.
J Clin Invest 92, 99-104.
Lee JE, Hillier SC & Knoderer CA (2008). Use of sildenafil to facilitate weaning from inhaled nitric
oxide in children with pulmonary hypertension following surgery for congenital heart disease. J
Intensive Care Med 23, 329-334.
Levin DL (1978). Morphologic analysis of the pulmonary vascular bed in congenital left-sided
diaphragmatic hernia. J Pediatr 92, 805-809.
Li F, Xia W, Yuan S & Sun R (2009). Acute inhibition of Rho-kinase attenuates pulmonary hypertension
in patients with congenital heart disease. Pediatr Cardiol 30, 363-366.
Lipkin PH, Davidson D, Spivak L, Straube R, Rhines J & Chang CT (2002). Neurodevelopmental and
medical outcomes of persistent pulmonary hypertension in term newborns treated with nitric
oxide. J Pediatr 140, 306-310.
Liu KS, Tsai FC, Huang YK, Wu MY, Chang YS, Chu JJ & Lin PJ (2009). Extracorporeal life support: a
simple and effective weapon for postcardiotomy right ventricular failure. Artif Organs 33, 504-
508.
Liu Y, Suzuki YJ, Day RM & Fanburg BL (2004). Rho kinase-induced nuclear translocation of
ERK1/ERK2 in smooth muscle cell mitogenesis caused by serotonin. Circ Res 95, 579-586.
Lopez-Ilasaca M (1998). Signaling from G-protein-coupled receptors to mitogen-activated protein
(MAP)-kinase cascades. Biochem Pharmacol 56, 269-277.
Maeda A, Yano T, Itoh Y, Kakumori M, Kubota T, Egashira N & Oishi R (2010). Down-regulation of
RhoA is involved in the cytotoxic action of lipophilic statins in HepG2 cells. Atherosclerosis
208, 112-118.
74
Maekawa M, Ishizaki T, Boku S, Watanabe N, Fujita A, Iwamatsu A, Obinata T, Ohashi K, Mizuno K &
Narumiya S (1999). Signaling from Rho to the actin cytoskeleton through protein kinases ROCK
and LIM-kinase. Science 285, 895-898.
McMurtry IF, Bauer NR, Fagan KA, Nagaoka T, Gebb SA & Oka M (2003). Hypoxia and Rho/Rho-
kinase signaling. Lung development versus hypoxic pulmonary hypertension. Adv Exp Med Biol
543, 127-137.
McNamara PJ, Murthy P, Kantores C, Teixeira L, Engelberts D, van Vliet T, Kavanagh BP & Jankov RP
(2008). Acute vasodilator effects of Rho-kinase inhibitors in neonatal rats with pulmonary
hypertension unresponsive to nitric oxide. Am J Physiol Lung Cell Mol Physiol 294, L205-213.
Mercier O, Sage E, de Perrot M, Tu L, Marcos E, Decante B, Baudet B, Herve P, Dartevelle P, Eddahibi
S & Fadel E (2009). Regression of flow-induced pulmonary arterial vasculopathy after flow
correction in piglets. J Thorac Cardiovasc Surg 137, 1538-1546.
Meyrick B & Reid L (1981). The effect of chronic hypoxia on pulmonary arteries in young rats. Exp
Lung Res 2, 257-271.
Meyrick B & Reid L (1982). Normal postnatal development of the media of the rat hilar pulmonary
artery and its remodeling by chronic hypoxia. Lab Invest 46, 505-514.
Michelakis E, Tymchak W, Lien D, Webster L, Hashimoto K & Archer S (2002). Oral sildenafil is an
effective and specific pulmonary vasodilator in patients with pulmonary arterial hypertension:
comparison with inhaled nitric oxide. Circulation 105, 2398-2403.
Mohseni-Bod H & Bohn D (2007). Pulmonary hypertension in congenital diaphragmatic hernia. Semin
Pediatr Surg 16, 126-133.
Murphy JD, Rabinovitch M, Goldstein JD & Reid LM (1981). The structural basis of persistent
pulmonary hypertension of the newborn infant. J Pediatr 98, 962-967.
Murthy KS (2006). Signaling for contraction and relaxation in smooth muscle of the gut. Annu Rev
Physiol 68, 345-374.
Nagaoka T, Fagan KA, Gebb SA, Morris KG, Suzuki T, Shimokawa H, McMurtry IF & Oka M (2005).
Inhaled Rho kinase inhibitors are potent and selective vasodilators in rat pulmonary
hypertension. Am J Respir Crit Care Med 171, 494-499.
Nagaoka T, Morio Y, Casanova N, Bauer N, Gebb S, McMurtry I & Oka M (2004). Rho/Rho kinase
signaling mediates increased basal pulmonary vascular tone in chronically hypoxic rats. Am J
Physiol Lung Cell Mol Physiol 287, L665-672.
Nakagawa O, Fujisawa K, Ishizaki T, Saito Y, Nakao K & Narumiya S (1996). ROCK-I and ROCK-II,
two isoforms of Rho-associated coiled-coil forming protein serine/threonine kinase in mice.
FEBS Lett 392, 189-193.
Namachivayam P, Theilen U, Butt WW, Cooper SM, Penny DJ & Shekerdemian LS (2006). Sildenafil
prevents rebound pulmonary hypertension after withdrawal of nitric oxide in children. Am J
Respir Crit Care Med 174, 1042-1047.
75
The Neonatal Inhaled Nitric Oxide Study Group (NINOS) (1997). Inhaled nitric oxide and hypoxic
respiratory failure in infants with congenital diaphragmatic hernia. Pediatrics 99, 838-845.
The Neonatal Inhaled Nitric Oxide Study Group (2000). Inhaled nitric oxide in term and near-term
infants: neurodevelopmental follow-up of the neonatal inhaled nitric oxide study group
(NINOS). J Pediatr 136, 611-617.
Nishimaru K, Tanaka Y, Tanaka H & Shigenobu K (2003). Inhibition of agonist-induced positive
inotropy by a selective Rho-associated kinase inhibitor, Y-27632. J Pharmacol Sci 92, 424-427.
Nwariaku FE, Rothenbach P, Liu Z, Zhu X, Turnage RH & Terada LS (2003). Rho inhibition decreases
TNF-induced endothelial MAPK activation and monolayer permeability. J Appl Physiol 95,
1889-1895.
Ostman A, Thyberg J, Westermark B & Heldin CH (1992). PDGF-AA and PDGF-BB biosynthesis:
proprotein processing in the Golgi complex and lysosomal degradation of PDGF-BB retained
intracellularly. J Cell Biol 118, 509-519.
Parker TA, Roe G, Grover TR & Abman SH (2006). Rho kinase activation maintains high pulmonary
vascular resistance in the ovine fetal lung. Am J Physiol Lung Cell Mol Physiol 291, L976-982.
Pearson DL, Dawling S, Walsh WF, Haines JL, Christman BW, Bazyk A, Scott N & Summar ML
(2001). Neonatal pulmonary hypertension--urea-cycle intermediates, nitric oxide production, and
carbamoyl-phosphate synthetase function. N Engl J Med 344, 1832-1838.
Porchia F, Papucci M, Gargini C, Asta A, De Marco G, Agretti P, Tonacchera M & Mazzoni MR (2008).
Endothelin-1 up-regulates p115RhoGEF in embryonic rat cardiomyocytes during the
hypertrophic response. J Recept Signal Transduct Res 28, 265-283.
Pourmahram GE, Snetkov VA, Shaifta Y, Drndarski S, Knock GA, Aaronson PI & Ward JP (2008).
Constriction of pulmonary artery by peroxide: role of Ca2+ release and PKC. Free Radic Biol
Med 45, 1468-1476.
Rabinovitch M (1989). New developments in the pathogenesis of pulmonary hypertension in the
newborn and child. Acta Paediatr Jpn 31, 631-640.
Rabinovitch M, Gamble W, Nadas AS, Miettinen OS & Reid L (1979). Rat pulmonary circulation after
chronic hypoxia: hemodynamic and structural features. Am J Physiol 236, H818-827.
Rabinovitch M, Gamble WJ, Miettinen OS & Reid L (1981). Age and sex influence on pulmonary
hypertension of chronic hypoxia and on recovery. Am J Physiol 240, H62-72.
Rame JE (2009). Pulmonary hypertension complicating congenital heart disease. Curr Cardiol Rep 11,
314-320.
Rattan R, Giri S, Singh AK & Singh I (2006). Rho/ROCK pathway as a target of tumor therapy. J
Neurosci Res 83, 243-255.
Rattan S & Patel CA (2008). Selectivity of ROCK inhibitors in the spontaneously tonic smooth muscle.
Am J Physiol Gastrointest Liver Physiol 294, G687-693.
76
Riento K & Ridley AJ (2003). Rocks: multifunctional kinases in cell behaviour. Nat Rev Mol Cell Biol 4,
446-456.
Rubin LJ, Badesch DB, Barst RJ, Galie N, Black CM, Keogh A, Pulido T, Frost A, Roux S, Leconte I,
Landzberg M & Simonneau G (2002). Bosentan therapy for pulmonary arterial hypertension. N
Engl J Med 346, 896-903.
Sakai H (2004). Possible structure and function of the extra C-terminal sequence of pyruvate kinase from
Bacillus stearothermophilus. J Biochem 136, 471-476.
Sakamoto K, Hori M, Izumi M, Oka T, Kohama K, Ozaki H & Karaki H (2003). Inhibition of high K+-
induced contraction by the ROCKs inhibitor Y-27632 in vascular smooth muscle: possible
involvement of ROCKs in a signal transduction pathway. J Pharmacol Sci 92, 56-69.
Sartori C, Allemann Y, Trueb L, Delabays A, Nicod P & Scherrer U (1999). Augmented vasoreactivity
in adult life associated with perinatal vascular insult. Lancet 353, 2205-2207.
Sasaki Y, Suzuki M & Hidaka H (2002). The novel and specific Rho-kinase inhibitor (S)-(+)-2-methyl-
1-[(4-methyl-5-isoquinoline)sulfonyl]-homopiperazine as a probing molecule for Rho-kinase-
involved pathway. Pharmacol Ther 93, 225-232.
Sawada N, Itoh H, Yamashita J, Doi K, Inoue M, Masatsugu K, Fukunaga Y, Sakaguchi S, Sone M,
Yamahara K, Yurugi T & Nakao K (2001). cGMP-dependent protein kinase phosphorylates and
inactivates RhoA. Biochem Biophys Res Commun 280, 798-805.
Schermuly RT, Dony E, Ghofrani HA, Pullamsetti S, Savai R, Roth M, Sydykov A, Lai YJ, Weissmann
N, Seeger W & Grimminger F (2005). Reversal of experimental pulmonary hypertension by
PDGF inhibition. J Clin Invest 115, 2811-2821.
Short BL (2005). The effect of extracorporeal life support on the brain: a focus on ECMO. Semin
Perinatol 29, 45-50.
Snedecor GW, Cochran, W.G. (1968). Statistical Methods.
Soll RF (2009). Inhaled nitric oxide in the neonate. J Perinatol 29 Suppl 2, S63-67.
Somlyo AP, Wu X, Walker LA & Somlyo AV (1999). Pharmacomechanical coupling: the role of
calcium, G-proteins, kinases and phosphatases. Rev Physiol Biochem Pharmacol 134, 201-234.
Sugiyama A, Yatomi Y, Takahara A, Satoh Y & Hashimoto K (2002). Cardiac effects of a selective rho-
associated kinase inhibitor, Y-27632, assessed in canine isolated, blood-perfused heart
preparations. Jpn J Pharmacol 88, 359-361.
Tanaka Y, Hayashi T, Kitajima H, Sumi K & Fujimura M (2007). Inhaled nitric oxide therapy decreases
the risk of cerebral palsy in preterm infants with persistent pulmonary hypertension of the
newborn. Pediatrics 119, 1159-1164.
Thibeault DW, Truog WE & Ekekezie, II (2003). Acinar arterial changes with chronic lung disease of
prematurity in the surfactant era. Pediatr Pulmonol 36, 482-489.
77
Thumkeo D, Shimizu Y, Sakamoto S, Yamada S & Narumiya S (2005). ROCK-I and ROCK-II
cooperatively regulate closure of eyelid and ventral body wall in mouse embryo. Genes Cells 10,
825-834.
Tourneux P, Chester M, Grover T & Abman SH (2008). Fasudil inhibits the myogenic response in the
fetal pulmonary circulation. Am J Physiol Heart Circ Physiol 295, H1505-1513.
Uehata M, Ishizaki T, Satoh H, Ono T, Kawahara T, Morishita T, Tamakawa H, Yamagami K, Inui J,
Maekawa M & Narumiya S (1997). Calcium sensitization of smooth muscle mediated by a Rho-
associated protein kinase in hypertension. Nature 389, 990-994.
Utsunomiya H, Nakatani S, Okada T, Kanzaki H, Kyotani S, Nakanishi N, Kihara Y & Kitakaze M
(2009). A simple method to predict impaired right ventricular performance and disease severity
in chronic pulmonary hypertension using strain rate imaging. Int J Cardiol.
Walsh-Sukys MC (1993). Persistent pulmonary hypertension of the newborn. The black box revisited.
Clin Perinatol 20, 127-143.
Walsh-Sukys MC, Tyson JE, Wright LL, Bauer CR, Korones SB, Stevenson DK, Verter J, Stoll BJ,
Lemons JA, Papile LA, Shankaran S, Donovan EF, Oh W, Ehrenkranz RA & Fanaroff AA
(2000). Persistent pulmonary hypertension of the newborn in the era before nitric oxide: practice
variation and outcomes. Pediatrics 105, 14-20.
Weigand L, Sylvester JT & Shimoda LA (2006). Mechanisms of endothelin-1-induced contraction in
pulmonary arteries from chronically hypoxic rats. Am J Physiol Lung Cell Mol Physiol 290,
L284-290.
Wu-Wong JR, Chiou WJ, Dickinson R & Opgenorth TJ (1997). Endothelin attenuates apoptosis in
human smooth muscle cells. Biochem J 328 ( Pt 3), 733-737.
Xue F, Zhang JJ, Qiu F, Zhang M, Chen XS, Li QG, Han LZ, Xi ZF & Xia Q (2007). Rho signaling
inhibitor, Y-27632, inhibits invasiveness of metastastic hepatocellular carcinoma in a mouse
model. Chin Med J (Engl) 120, 2304-2307.
Xue Q, Ducsay CA, Longo LD & Zhang L (2008). Effect of long-term high-altitude hypoxia on fetal
pulmonary vascular contractility. J Appl Physiol 104, 1786-1792.
Yamboliev IA, Hedges JC, Mutnick JL, Adam LP & Gerthoffer WT (2000). Evidence for modulation of
smooth muscle force by the p38 MAP kinase/HSP27 pathway. Am J Physiol Heart Circ Physiol
278, H1899-1907.
Yi M, Jankov RP, Belcastro R, Humes D, Copland I, Shek S, Sweezey NB, Post M, Albertine KH, Auten
RL & Tanswell AK (2004). Opposing effects of 60% oxygen and neutrophil influx on
alveologenesis in the neonatal rat. Am J Respir Crit Care Med 170, 1188-1196.
Yi SL, Kantores C, Belcastro R, Cabacungan J, Tanswell AK & Jankov RP (2006). 8-Isoprostane-
induced endothelin-1 production by infant rat pulmonary artery smooth muscle cells is mediated
by Rho-kinase. Free Radic Biol Med 41, 942-949.
78
Zhai FG, Zhang XH & Wang HL (2009). Fluoxetine protects against monocrotaline-induced pulmonary
arterial hypertension is relevant to induction of apoptosis and up-regulation of Kv1.5 channels in
rats. Clin Exp Pharmacol Physiol.
Zhao L, Mason NA, Morrell NW, Kojonazarov B, Sadykov A, Maripov A, Mirrakhimov MM, Aldashev
A & Wilkins MR (2001). Sildenafil inhibits hypoxia-induced pulmonary hypertension.
Circulation 104, 424-428.
Ziino AJ, Ivanovska J, Belcastro R, Kantores C, Xu EZ, Lau M, McNamara PJ, Tanswell AK & Jankov
RP (2010). Effects of rho-kinase inhibition on pulmonary hypertension, lung growth, and
structure in neonatal rats chronically exposed to hypoxia. Pediatr Res 67, 177-182.