changes in the structure-function relationship of elastin and its impact on the proximal pulmonary...
Post on 14-Nov-2023
0 Views
Preview:
TRANSCRIPT
Changes in the structure-function relationship of elastin and its impact on the proximal pulmonary arterial mechanics of hypertensive calves Running Head: Elastin mechanics in pulmonary hypertension
Steve Lammers1, Phil Kao1, H. Jerry Qi1, Kendall Hunter2, Craig Lanning2, Joseph Albietz3, Stephen Hofmeister3, Robert Mecham4, Kurt R. Stenmark3, Robin Shandas1,2
(1) Mechanical Engineering
University of Colorado
Boulder, CO
(2) Dept. of Pediatric Cardiology
University of Colorado Health Sciences
Denver, CO
(3) Department of Pediatrics
Developmental Lung Biology Laboratory
University of Colorado Health Sciences
Denver, Colorado
(4) Dept. of Biology and Biomedical Sciences
Washington University
St. Louis, MO
Articles in PresS. Am J Physiol Heart Circ Physiol (July 25, 2008). doi:10.1152/ajpheart.00127.2008
Copyright © 2008 by the American Physiological Society.
1
Address for Correspondence:
Robin Shandas, Ph.D. Professor Center for Bioengineering University of Colorado 13123 E. 16th Avenue, B100 Aurora, CO 80045 Robin.shandas@uchsc.edu Phone: (720) 777 2586 Fax: (720) 777 4056
2
Abstract
Extracellular matrix remodeling has been proposed as one mechanism by which proximal
pulmonary arteries stiffen during pulmonary arterial hypertension (PAH). Although some
attention has been paid to the role of collagen and metallomatrix proteins in affecting vascular
stiffness, much less work has been performed on changes in elastin structure-function
relationships in PAH. Such work is warranted given the importance of elastin as the structural
protein primarily responsible for the passive elastic behavior of these conduit arteries. Here, we
study structure-function relationships of fresh arterial tissue and purified arterial elastin from the
main, left and right pulmonary artery branches of normotensive and hypoxia-induced pulmonary
hypertensive neonatal calves. PAH resulted in an average 81% and 72% increase in stiffness of
fresh and digested tissue respectively. Increase in stiffness appears most attributable to elevated
elastic modulus, which increased 46% and 65% respectively for fresh and digested tissue.
Comparison between fresh and digested tissues shows that, at 35% strain, a minimum of 48% of
the arterial load is carried by elastin, and a minimum of 43% of the change in stiffness of arterial
tissue is due to the change in elastin stiffness. Analysis of the stress-strain behavior revealed that
PAH causes an increase in the strains associated with the physiologic pressure range but had no
effect on the strain of transition from elastin-dominant to collagen-dominant behavior. These
results indicate that mechanobiological adaptations of the continuum and geometric properties of
elastin, in response to PAH, significantly elevate the circumferential stiffness of proximal
pulmonary arterial tissue.
Key Words: pulmonary hypertension, elastic modulus, stiffness, vascular remodeling
3
Introduction
Pulmonary arterial hypertension (PAH) in neonates, infants and children is a progressive
condition marked by substantial vascular remodeling of the distal pulmonary vasculature, which
increases pulmonary vascular resistance (PVR) and pulmonary arterial pressure. PVR
measurement has been the standard diagnostic for evaluating both the significance of PAH and
the extent of vascular response to therapies. However, PVR is an inherently limited diagnostic in
that it ignores pulmonary vascular stiffness (PVS), an especially important omission given the
inherently pulsatile nature of cardiac function and the importance of robust ventriculo-vascular
coupling in maintaining hemodynamic efficiency through the pulmonary vasculature. In fact,
many studies of vascular function in systemic hypertension are documenting the substantial role
played by the elastic proximal arteries in maintaining systemic vascular hemodynamic efficiency
and reducing cardiac workload. Several investigators have shown the significant mechanical
advantages conveyed by the elasticity of systemic conduit arteries in reducing overall hydraulic
impedance and cardiac workload (29, 32, 37, 38). Other authors have correlated proximal artery
stiffness and cardiovascular mortality for patients with systemic hypertension (5, 13, 28).
Although less work has been done regarding pulmonary artery (PA) elasticity in PAH, several
recent animal studies are beginning to address this topic. In particular, recent work by Kobs and
Chesler used fresh artery material testing to correlate increased collagen and elastin content with
elevated elastic moduli for the collagen and elastin dominant regions of the stress-strain curve
respectively(26).
In addition, several clinical studies have shown that increased PVS is correlated with
patient mortality (12, 18, 31, 43) and can account for as much as 30% to 40% of the increased
load on the heart (40) due to elevated vascular hydraulic impedance and right ventricular
4
afterload. Remodeling of the extra-cellular matrix (ECM) in particular appears to be an
important aspect of PVS and a number of studies have examined various biological mechanisms
including inflammatory factors, upregulation of proliferative catalysts, and phenotypic changes
in resident cells (2-4, 6, 17, 20-24, 40, 41, 44). Other studies have shown increased collagen
content and vascular tone in stiffer arteries (7, 11, 14, 19, 21, 27, 34, 35). In elastin specific
studies, elastolytic activity has been shown to increase during PAH (33), and inhibition of this
pathway by the serine elastase inhibitor elafin mitigates hypoxia-induced PAH (46). In recent
work from our group coupling a novel orthotropic, hyperelastic, microstructural model of the PA
wall to biomechanical studies of PAs from normotensive and hypertensive rats, we suggested
that increased ECM structural protein crosslinking may be one mechanism by which these
vessels stiffen (47, 48). The next step in addressing this hypothesis is to evaluate
experimentally whether the increased stiffness seen in hypoxia-induced PAH can be attributable
to increased stiffness of the structural protein matrix. Given that elastin is the ECM protein
largely responsible for vascular elasticity, we evaluate here in a well-established PAH neonatal
calf model the role of elastin in modulating the stiffness of upstream PA vessels.
In this study, we hypothesize that changes in the functional mechanical properties of
elastin is one of the primary causes of the increased stiffness seen in the proximal PAs due to
hypoxia-induced PAH. To test this hypothesis, we examined the biomechanics and structure of
normotensive and hypertensive neonatal calf proximal PAs and their associated elastin tissue.
5
Materials and methods
Animal model
All studies were performed after approval by institutional animal care and use
committees. Arterial tissues from 3 normotensive and 6 hypertensive male Holstein calves (70-
110lb) were used. Hypertension was induced by hypobaric hypoxia, 2wks, 430 mmHg [4600 m
equivalent air pressure]. Hypoxic animals were sacrificed at 430 mmHg pressure after 14 days at
hypoxic conditions. All animals were studied and sacrificed at 15 ± 1-2 days of age. PA
pressures were obtained with a 5-French Swan-Ganz or Millar catheter, positioned in the main
PA. After sacrifice the right, left and main PAs (RPA, LPA, MPA) were excised, stored in
nutrient balanced medium (4 ºC). Testing was conducted within 24 hours of sacrifice, material
properties of fresh tissues were unchanged for tests conducted up to 4 days post sacrifice.
Geometric and material property results were calculated using 3 control and 6
hypertensive tissues for the LPA and MPA. Two hypertensive RPA tissues were too small and
irregularly shaped for stress-strain testing; therefore 3 control and 4 hypertensive RPA tissues
were used. We were also unable to accurately measure the pulmonary arterial pressure for one
hypertensive animal. Due to this, 3 control and 5 hypertensive LPA and MPA and 3 control and
4 hypertensive RPA tissues were used for all material property comparisons made at physiologic
pressure/strain values.
Tissue dissection and processing
Arteries were inspected for holes, tears, branch points and localized thickening or other
anomalies that may adversely affect test results. Loose connective tissue was removed, and
gross anatomical measurements of diameter (1-distal, 1-proximal) and wall thickness (4-distal, 4-
6
proximal) were obtained with digital calipers prior to axial bisection, see figure 1.
Circumferential rectangular sections (~8mm x 20mm) were taken for subsequent material
testing. Biopsy samples were taken for histological analysis, three each in the longitudinal and
circumferential directions.
Materials testing
Fresh tissue stress-strain data was acquired with an MTS, Insight 2 (MTS Systems
Corporation, Eden Prairie, MN) material testing system, equipped with an ancillary
environmental chamber and either 5N or 2kN load cell, depending on the maximum expected
load for each test, figure 2. Stress-strain tests were conducted in Calcium and Magnesium-free
NaCl-PBS buffer (.01 mol/L, ionic str. 0.15, pH 7.4) 36ºC. Sample width, thickness and gage
length were measured using digital calipers. Stress-strain properties remained consistent for
tissue tests performed up to three days post sacrifice.
Tissues were preconditioned by ten full extension-relaxation cycles before data were
taken. The strain rate for all mechanical tests was 10% strain per second. In this study, force
and stress data refer to the loading region of the stress-strain curve. In an effort to avoid damage
that may affect elastin-only material tests, tissues were stretched until the collagen-dependent
strain-stiffening response became fully developed, typically 60 – 80% strain, figure 3. Elastin
tissue tests were conducted in the same manner as that outlined for fresh arteries, but with a 2N
or 5N load cell. Elastin samples were tested at strains ranging from 60 to 100% at 10%
increments or until failure. Data processing was conducted using custom-written software
(Matlab® R2006a, The Math Works, Inc., Natick, MA).
7
Tissue digestion using formic acid – CNBr solution
After fresh artery material testing, tissues were processed into elastin-only scaffolds using
the CNBr-formic acid-digestion procedure outlined by Lu et al (30). Briefly, fresh arteries were
submerged in a 70% formic acid, 50 mg/mL Cyanogen Bromide (CNBr) solution and gently
stirred for 19 hours at room temperature followed by 1 hour at 60ºC. The samples were then
boiled for 10 min. to remove any residual CNBr. The digestion solution was then decanted and
the tissue was rinsed with distilled water.
CNBr-formic acid-digestion was chosen for elastin purification due to its effectiveness
for removing non-elastin components from arterial tissues. Other common elastin purification
procedures using hot alkali or autoclaving were rejected due to possible network fragmentation
and incomplete elastin purification respectively (15).
Amino acid analysis was performed on LPA elastin samples (n=7) to determine the
effectiveness of the digestion procedure. After digestion, the samples retain formic acid and
subsequent material testing showed strong pH dependence. NaOH titration was therefore used to
raise the pH from 2-3 to 7.4. After titration, samples were stored in NaCl-PBS buffer and were
tested within 2 weeks of animal sacrifice. Elastin mechanical properties were unchanged for
tests conducted up to one month post sacrifice.
Histology and elastin area fraction
Biopsies were fixed in 10% buffered formalin, wax embedded, sectioned and stained for
elastin using Verhoeff’s Van Gieson. Bright-field photomicrographs were taken with a Nikon
TE-200 (Nikon Instruments Inc., Melville, NY) microscope (40-X magnification, SPOT RT-900
camera [Diagnostic Instruments Inc., Sterling Heights, MI]). Elastin area fraction was
8
determined using custom software (Matlab® R2006a Image Processing Toolbox, The Math
Works, Inc., Natick, MA).
Calculations
Fresh artery Cauchy stress (σfresh) was calculated with the assumption of
incompressibility applied to the width (W) and thickness (T) directions to account for changes in
cross-sectional area as a function of engineering strain (ε).
WTF
fresh =σ elast
elast AWTF0=σ (1)
( ) νε −+= 10TT ( ) νε −+= 10WW (2)
0
0
LLL −=ε (3)
Where F is the applied force and L is the loaded sample length in the direction of applied load.
T0, W0 and L0 are the initial thickness, width and length respectively, Aelast is the area fraction of
elastin and υ is Poisson’s ratio (0.5 for incompressible tissue). Due to the layered structure of the
fenestrated elastic sheets, stresses for the digested elastin samples (σelast) were calculated with the
condition of incompressibility applied to the width direction only. To facilitate modulus (Ε)
calculations, stress-strain data for fresh and elastin samples were fit with 9th and 4th order
polynomials respectively. The 9th and 4th order polynomials were determined to be the lowest
order polynomials necessary to achieve an average squared correlation coefficient R2avg >=0.995
for all fresh and elastin datasets respectively.
9
εσ
dd=Ε (5)
Stiffness (Φ) is the derivative of the width-normalized force (Fn: force divided by current
width) by strain, and as such, stiffness is dependent upon thickness geometry and represents the
extensive equivalent of elastic modulus.
( ) ( )( )εεεε nF
dd
WF
dd =⎟⎟
⎠
⎞⎜⎜⎝
⎛=Φ (6)
The condition of incompressibility was applied to the stiffness calculation to account for any
variation in width as a function of imposed strain. Fn data were fit to polynomials in the same
manner as was used for the stress. Unless otherwise noted, all results for the material parameters
(Ε, Φ) were calculated at a strain of 35%, so that tissues could be compared. Strains higher than
35% resulted in one or more of the stress-strain curves extending into the collagen-dominant,
strain-stiffening region. At strains greater then 35%, any comparison between fresh and elastin
stress-strain data would be complicated by the active loading of collagen. Since this collagen
component cannot be removed from the fresh artery dataset, any comparison of the mechanical
properties made at strains greater then 35% would include collagen and therefore not allow for
the direct comparison of elastin mechanical property changes from the fresh to digested state.
Lame’s equation for stress in thick-walled tubes (7) was used to determine the strains that
correspond to the measured physiologic pressures.
( )( )( ) 22
22
rTrTrrPi
L −+++
=σ , ( )ε+= 10rr (7)
Lame’s equation was equated to the polynomial stress-strain function and solved iteratively for
the strains that correspond to the in vivo measured systolic, diastolic and mean pressures (Pi); r
and r0 are the internal radii of the artery in the loaded and initial state respectively. The
10
estimated physiologic strains were then used to calculate the systolic and diastolic moduli using
equation 5.
Curvature (κ) of the stress-strain curve was used to determine the onset of collagen
engagement, figure 4.
( ) 2321 σ
σκ′+
′′= (8)
The 2nd order derivative in the numerator of the curvature equation led to large variances when
calculated from the polynomial fit to the original stress-strain data. We therefore applied a zero-
phase, low-pass, elliptic digital filter to smooth the data. A new 9th order polynomial was then fit
to the filtered data, resulting in reduced curvature variance.
Average pre-strain-stiffening curvature (κPSS) was calculated for the strain range (εPSS)
between εL and εH, where εL equals 20% strain and εH equals the strain associated with maximum
curvature minus 20% strain, figure 4. εL and εH were defined in this way so that any curvature
associated with the low-strain loading region or high-strain strain-stiffening region would not
influence the κPSS value. Transition strain (εtrans) was then determined by the relationship:
100H
trans =κ PSSH κκ −= max (9)
such that εtrans is associated with the onset of curvature elevation. εtrans results compare
favorably to those previously published using both experimental(36) as well as Lorentz
distribution functions(45, 49). Stress-strain plots of elastin tissue do not exhibit curvature
elevation behavior, and since strain-stiffening is associated with collagen engagement, we
defined εtrans as the strain at which collagen begins to carry load. Strains below this value fall
within the elastin-dominant region of the stress-strain curve, A in figure 4, while strains which
are greater fall within the transitional or collagen-dominant region, B. We further defined the
11
collagen dominant region (εcd) as those strains which result in a fresh artery modulus greater than
ten times the artery modulus calculated within the elastin dominant region at a strain of 35%.
While this is an arbitrary definition for collagen dominance it seemed logical to suggest that
collagen is the dominant load bearing structural protein when at least 90% of the material
modulus can be attributed to collagen.
Equation (10) defines the percent of the fresh tissue load that is carried by elastin (%Fn-C,
%Fn-H) and the percent of the increased load, due to PAH, which is attributable to the increased
stiffness of elastin (%Fn-e,f), calculated at a strain of 35%.
⎟⎟⎠
⎞⎜⎜⎝
⎛=
−
−−
Cfn
CenCn F
FF
,
,%% ⎟⎟⎠
⎞⎜⎜⎝
⎛=
−
−−
Hfn
HenHn F
FF
,
,%% ⎟⎟⎠
⎞⎜⎜⎝
⎛
−−
=−−
−−−
CfnHfn
CenHenfen FF
FFF
,,
,,, %%
Fn-f,C , Fn-f,H : Fn, fresh tissue (control, hypertensive).
Fn-e,C , Fn-e,H : Fn, elastin tissue (control , hypertensive).
(10)
Fn-C and Fn-H were similarly calculated at systolic and diastolic strains to determine the percent
load carrying capacity of elastin at physiologic strains.
P-values refer to the probability associated with the one-tail, two-sample equal variance,
Student’s t-test. Results were deemed statistically significant for P-values<=0.05. All error bars
represent one standard deviation above and below the mean. Standard deviations (S) were
calculated using the “n-1” method. In all curve fitting, the average of the squared correlation
coefficient was deemed statistically significant for R2avg >=0.995.
12
Results
Morphology
PAH resulted in an increase in vessel wall thickness by 30% (S=12%, P=0.02), 28%
(S=11%, P=0.04) and 26% (S=8%, P=0.03,) for the RPA, LPA and MPA respectively, figure 5.
There was no statistically significant change in the internal diameter as a result of hypertension.
PAH also caused a decrease in the area fraction of elastin by 17% (S=2%, P=0.03), 16% (S=2%,
P=0.01) and 16% (S=3%, P=0.03) for the RPA, LPA and MPA respectively, figure 5. The
elastin content factor (ECF) is the product of the elastin area fraction and tissue thickness and is
representative of the volume of elastin in a given tissue cross section. The increase in ECF,
resulting from PAH, was calculated to be 7.6% (S=3.1%), 7.7% (S=3.1%) and 5.5% (S=2.0%)
for the RPA, LPA and MPA respectively, average ECF=6.9% (S=1.2%).
Physiology
Average systolic/diastolic pressures were 45/18 mmHg (S=12/7 mmHg) and 146/71 mmHg
(S=29/18 mmHg) for control and hypoxic populations respectively. Control and hypoxic mean
pulmonary pressures were 31 mmHg (S=12 mmHg) and 106 mmHg (S=16 mmHg) respectively.
We were unable to collect accurate diameter data, for all tested tissues; therefore, the strain at
systole and diastole were calculated using Lame’s equation (7) with average unloaded internal
radii calculated for each MPA, RPA and LPA; measured from 4 control and 11 hypertensive
tissues. The average systolic/diastolic strains for the PAs were 59% (S=10%) / 34% (S=6%)
and 72% (S=13%) / 53% (S=11%) for the control and hypoxic populations respectively. The
average strain for the mean pulmonary pressures were 47% (S=8%) and 65% (S=12%) for the
control and hypoxic populations respectively. The average transition strain was unchanged by
13
PAH, 49% (S=8%) for control and 51% (S=9%) for hypertensive tissues (P=0.29). Transition
strain values are comparable to the strain corresponding with the onset of collagen engagement
published by Zulliger (49). The strain associated with the onset of collagen-dominance was
calculated to be 69% (S=7%) and 74% (S=8%) for the control and hypoxic populations
respectively.
Mechanical properties of fresh tissue
At 35% strain,the average increase in stiffness, due to PAH, was 72% (S=30%, P=0.01),
107% (S=56%, P=0.01) and 63% (S=14%, P=0.01) for the RPA, LPA and MPA respectively,
figure 6. The overall average increase in stiffness was 81% (S=23%, P<<0.05). PAH also
caused an in the increase in modulus of PA tissues by 28% (S=7%, P=0.04), 45% (S=23%,
P=0.10) and 65% (S=18%, P=0.02) for the RPA, LPA and MPA respectively. The average
overall increase in fresh tissue modulus was 46% (S=18%, P=0.02). Average stiffness values at
physiologic strains are shown in figure 7, and comparisons between physiologic stiffness values
are detailed in table 1.
Mechanical properties of purified arterial elastin
At 35% strain PAH resulted in an increase in the stiffness of the elastin by 57% (S=19%,
P=0.04), 109% (S=68%, P=0.03) and 50% (S=17%, P=0.05) for the RPA, LPA and MPA
respectively, figure 8. The overall average increase in the stiffness of elastin was 72% (S=33%,
P=0.01). The modulus of elastin increased by 34% (S=7%, P=0.04), 88% (S=43%, P=0.01) and
73% (S=36%, P=0.07) for the RPA, LPA and MPA respectively. The overall average increase in
the modulus of elastin was 65% (S=28%, P<<0.05). Elastin stiffness at physiologic pressure is
detailed in figure 7 and table 1. Amino acid analysis confirmed that CNBr-formic acid digestion
14
resulted in elastin tissue samples of high purity(25), as evidenced by the high number of residues
per 1000 for alanine (227, S=20), valine (127, S=6) and glycine (342, S=16), along with the lack
of methionine and hydroxylysine residues (trace) and the low concentration of hydroxyproline
(14, S=5).
Average values for %Fn-C and %Fn-H are 51% (S=16%, P=0.02) and 48% (S=13%,
P=0.003) respectively, meaning that at a minimum, roughly half of the load applied to the fresh
arteries is carried by elastin for both control and hypertensive conditions at a strain of 35%.
Also, %Fn-e,f indicates that the change in the stiffness of the elastin accounts for an average of
43% (S=10%, P=0.003) of the change in the stiffness of the fresh tissue as a result of
hypertension. Changes in elastin load carrying capacity at physiologic strains are detailed in
table 1.
Discussion
Several key issues arise from this study. First, both the physiologic pressure and PA
stiffness elevation for the hypoxia-induced neonatal calf model mimic the changes we have seen
in the human (12), and confirm the value of this model for studying PA stiffness and impedance
changes in PAH. Second, the increases in stiffness appear attributable to a significant extent on
material rather than purely geometric factors. Third, the changes in material modulus due to
PAH appear to be significantly attributable to changes in elastin modulus specifically. Fourth,
the physiologic tissue strain at diastolic pressure is largely dependent on the stiffness of elastin.
Lastly, a significant component of the mechanical load for both normal and hypertensive
conditions continues to be carried by elastin. We comment on each of these issues below.
15
Use of the Neonatal Bovine Model
The normal and pathologic physiology of the bovine model more closely mimics that of
humans than that of the available rodent models. Humans and young calves both have similar
body mass, heart rate, blood pressure and vascular wall thickness. In addition, the cellular
composition of the proximal PA wall of the large mammals is similarly complex to humans,
incorporating numerous phenotypically distinct smooth muscle cell populations which rapidly
proliferate during PAH (40, 41). For these reasons and the fact that we have significant
experience with this model, we chose the hypoxic neonatal calf as the in vivo model for
understanding how the proximal PA stiffens during hypoxia-induced PAH.
Impact of PAH on physiologic strain
Hypoxic conditions successfully induced PAH as evidenced by the significant increase in
mean PA pressure, vascular wall thickness and PVS. Due to the stress-strain nonlinearity of
arterial tissue, the relative contribution of elastin and collagen is contingent upon the strains
associated with in vivo physiologic pressures. Our results indicate that the physiologic region
of the stress-strain curve bounds the transition strain, with 62% of the curve residing in the
elastin-dominant region and 38% in the transition region for the control population, figure 9.
Hypertension shifts the physiologic strain region to higher strain values, but has no effect on the
transition strain. The resulting diastolic strain of hypertensive tissues is roughly equal to the
transition strain, 53% and 50% respectively, and the systolic strain of 72% nearly equals the
strain associated with collagen-dominant stress-strain behavior (74% in PAH
tissues).Hypertensive stress-strain curves therefore begin at the transition strain and reside
entirely within the transition region. This bounding of the transition strain in control tissues and
16
the correlation of transition and diastolic strains for hypertensive tissues suggests that the
diastolic strain, and therefore baseline slope, of the stress-strain curve is set by the stiffness of
elastin, while the systolic strain incorporates collagen engagement.
At diastolic strain, PAH causes a 293% (ΦDias, Cont to PAH) increase in artery stiffness,
figure 7, table 1. Since diastolic strain resides within the elastin dominant region for control
tissues and at the transition strain for PAH tissues, this increase in diastolic stiffness is likely the
result of both increased elastin stiffness and the onset of collagen engagement. We calculate that
PAH causes a 173% (ΦDias, Cont to PAH) increase in diastolic elastin stiffness for digested samples.
The discrepancy in diastolic stiffness elevation between elastin and fresh tissue is a consequence
of the removal of non-elastin material during elastin purification, which will necessarily change
the mechanical properties of elastin between its natural and tested state. However, given that the
minimum percent diastolic load-carrying capacity of elastin is 61% (%Fn Dias, Cont) and 48% (%Fn
Dias, PAH) for the control and PAH tissues respectively, and that elastin stiffness values are
relatively strain independent, we feel confident in stating that the change in diastolic stiffness,
due to PAH, is predominately a result of an increase in elastin stiffness.
The significant strain stiffening response of the transitional region acts to limit the
maximum systolic strain at elevated pressure. Our data shows that PAH causes an increase in
both fresh tissue and purified elastin systolic stiffness by 510% and 123% (ΦSys, Cont to PAH)
respectively. By comparing the systolic and diastolic stiffness change from control to
hypertensive tissues (ΦSys, Cont to PAH to ΦDias, Cont to PAH), we see that the systolic stiffness
elevation of fresh tissue, resulting from PAH, is nearly double that of the diastolic stiffness
elevation, while the elastin stiffness elevation remains relatively constant. This is not surprising
given the linear nature of the elastin stress-strain curve compared to the highly non-linear fresh
17
tissue curve. This highly nonlinear behavior coupled with the elevated PAH physiologic strain
results in an increase in stiffness for control and PAH tissue from diastolic to systolic strain of
145% (ΦCont, Dias to Sys) and 278% (ΦPAH, Dias to Sys) respectively, while the more linear elastin
tissue only increased 39% and 14% for control and PAH tissues respectively. Also, the
minimum percent systolic load-carrying capacity of elastin is reduced from 48% (%Fn Sys, Cont)
for control tissues to 32% (%Fn Sys, PAH) for PAH tissues indicating that collagen carries more
load in the diseased state. However, these data also shows that elastin is an important load
carrying material even at PAH systolic strains. Increased systolic tissue stiffness is therefore due
to both elevated elastin stiffness as well as a higher degree of collagen engagement resulting
from the increase in systolic strain due to PAH.
While our results indicate that PAH causes PA tissues to operate at higher strains, the
elevated stiffness of the elastin dominant region mitigates this effect and maintains the
physiologic strain range within the transitional region. Due to the large strains associated with
control fresh tissues operating at PAH physiologic pressures we were unable to consistently
stretch the control fresh tissues to strains large enough to attain hypoxic pressure-load values
without risk of tissue damage. However, by projecting the fitted polynomial curves of control
fresh tissues, we estimate that the PAH diastolic pressure intersects the control fresh tissue curve
at a strain of ~73%. At these high strains, the compliance of arterial tissue is significantly
reduced due to elevated tissue modulus resulting from increased collagen loading. Therefore, the
elevated stiffness of the PAH elastin dominant region of the stress-strain curve maintains the
physiologic strains of PAH arterial tissues within the transition region of the stress-strain curve
by lowering the diastolic strain from ~73% to 53%. Without this increased stiffness, PAH PA
tissues would operate entirely within the high modulus, collagen dominant, region of the stress-
18
strain curve, which would result in a significant reduction of the Windkessel effect. This further
underlines the importance of understanding how elastin contributes to the mechanical properties
and morphology of PA tissue in response to PAH.
Pulmonary Vascular Stiffness and Elastin
Typically, modulus is calculated with a cross-sectional area determined from microscopic
analysis of arterial sections(8-10, 16, 27, 39, 42). This method assumes that the constituent
artery materials maintain homogeneity regardless of pathology or anatomical location. Since
stiffness calculations do not require this assumption, the 72% increase in elastin stiffness is an
independent result indicating that elastin carries substantially more load in the pathologic state.
However, the removal of non-elastin tissue during the digestion process results in experimentally
measured material properties that differ between the isolated elastin tissue and elastin in its
native state.
Individual elastic fibers are arranged in a network and bound together to form fenestrated
elastic sheets which surround the artery in concentric layers and work to uniformly distribute
arterial loads (38). While the individual elastic fibers do not have a linear stress-strain
relationship, network effects allow the resulting elastin tissue to obey Hooke’s law up to large
strains(45). The resulting elastic sheets, which are bound to non-elastin ECM components and
smooth muscle cells through glycoprotein and integrin bonds, imbue the artery with a Neo-
Hookean load-carrying elastin component that behaves in a near perfectly elastic manner(1).
Hypertensive adaptation of these intra-tissue bonding proteins is thought to play a role in the
development of increased arterial stiffness (2-4, 6, 20-22); however, during the CNBr digestion
process the elastin intra-tissue bonds are broken and all non-elastin material is extracted. In
addition, the removal of bulk, non-elastin, artery material eliminates many of the constraints
19
which resist the movement of elastin sheets relative to one another. The removal of both the
intra-tissue bonds and non-elastin material likely results in experimentally measured stiffness
and modulus values that are lower then those of the tissue in its native state. However, any
discrepancy between the experimentally-determined and native elastin stiffness should have little
impact on material property comparisons between control and hypertensive elastin tissues, since
both underwent the same digestion process. Due to this discrepancy between the experimentally
measured and native stiffness properties, %Fn-C and %Fn-H should be considered as the lower
bound for the fresh tissue load fraction carried by elastin and %Fn-e,f defines the minimum
fraction of increased load directly attributable to hypertensive elastin tissue. Hypertension,
therefore, causes a significant increase in the stiffness of the elastin material responsible for
carrying roughly half (%Fn-C, %Fn-H) of the arterial tissue load in the elastin dominant region, at a
minimum.
PVS is a function of both the intrinsic material property of modulus and the extrinsic
geometric consideration of thickness. Our data show a 46% and 28% average increase in fresh
tissue modulus and thickness respectively and an 81% average increase in fresh tissue stiffness.
For elastin tissues our data show a 65% and 6.9% average increase in modulus and ECF
respectively and a 72% average increase in stiffness. Since the width-normalized force, and
hence stiffness, scale linearly with changes in both modulus and thickness, it is evident that
modulus, rather than geometric tissue thickening, is the dominant factor in determining the
stiffness of hypertensive arterial and elastin tissues. Also, it is interesting to note that the
stiffness elevation predicted by our fresh tissue modulus and thickness data is 87%, which is
close to the measured stiffness increase of 81%, and the stiffness elevation predicted by our
20
increase in elastin modulus and ECF is 76%, which is close to the 72% average increase in
measured elastin stiffness.
Elastin Modulus
Our biomechanical tests show that hypertension causes an increase in the modulus of
both the fresh and elastin arterial tissues by an average of 46% and 65% respectively. This
increase in elastin modulus supports our thinking that one of the primary structural targets of
proximal vascular remodeling during hypoxia-induced PAH is arterial elastin. Changes in fresh
artery modulus are comparable to the 30% average increase in the modulus of the PAs in mice
published by Kobs et al (26, 27) and 40% decrease in compliance, identified as the threshold for
pediatric hypertension in humans, by Dyer et al (12).
The increased modulus of elastin, resulting from hypertension, suggests either a change
in elastin fibril modulus or a structural adaptation in fibril orientation / inter-elastin binding. The
turnover rate for collagen and elastin is low in healthy arteries, but vascular pathology upsets the
regulatory pathways that maintain this balance. In response to hypertension, the over expression
of both pro-inflammatory and proteinase-inhibitory molecules dramatically increases arterial
ECM synthesis (2, 23, 24). Although little is known about the ECM synthesis pathway of
hypertensive arterial tissue, (2, 40) the upregulation of the MMP-1 (matrix metalloproteinase -1)
inhibitor TIMP-1 (Tissue Inhibitor of Matrix Metalloproteinase 1) is one method by which ECM
synthesis may be enhanced during hypertension (23, 24). However, the ECM proteins
synthesized in response to hypertension have a three-dimensional architecture which is
functionally less optimal then those deposited during fetal development, and may play an
important role in determining the modulus of pathologic elastin tissue (2, 23, 24). More
21
experimentation is required to determine the underlying cause for the increase in elastin
modulus; this will be the topic of future study.
Limitations
Several limitations in these studies must be acknowledged. First, the tissue digestion
procedure may alter the mechanical properties of elastin through chemical attack or thermal
degradation, although no evidence of this was found in our studies or in the literature. Second,
the use of continuum mechanics for discontinuous materials will lead to some degree of error in
calculated mechanical properties due to simplifying assumptions; however, this should have little
impact on comparison of those properties. Third, uni-axial rather than fully biaxial testing was
performed. However, given that the objective of this study was not to investigate the anisotropic
behaviors of artery tissues, but rather to determine how such properties of fresh and digested
tissue samples change as a result of hypertension, the uni-axial test was deemed sufficient.
Conclusion
Via biomechanical testing of both fresh and digested elastin tissues of control and
hypoxia-induced pulmonary hypertensive animals, we have confirmed that vascular remodeling
results in a significant increase in the modulus and stiffness of both the fresh and elastin tissues
of the proximal PAs in the circumferential direction. We have further shown that, at 35% strain
a minimum 48% of the load imposed on fresh arterial tissue is carried by elastin, and that, at a
minimum, 43% of the change in stiffness of fresh arterial tissue is directly attributable to the
change in stiffness of the elastin component of those arteries. We have also shown that PAH
causes an increase in the strains associated with the physiologic pressure range but had no effect
on the strain of transition from elastin-dominant to collagen-dominant behavior. Stress-strain
22
behavior of fresh arterial tissues further revealed that the diastolic strain and baseline slope of the
stress-strain curve are determined by elastin mechanics, and the strain at systole becomes
increasingly dependent on collagen mechanics as a result of hypertension. The final conclusion
drawn from the above statements is that elastin is an important passive material for carrying the
load imposed on the proximal PAs at physiologic pressure ranges, and that the increase in
stiffness of elastin acts to maintain the physiologic strain range within the more elastin dependent
region of the stress-strain curve.
Acknowledgments
The authors would like to thank Dr. Conrad Stoldt for the use of laboratory equipment and
Colorado State University for providing access to their hypobaric chamber.
Sources of Funding
NIH P50HL84923
NIH T32HL072738
NIH K24HL081506
Disclosures
None
References
1. Aaron BB and Gosline JM. Elastin as a Random-Network Elastomer - a Mechanical and Optical Analysis of Single Elastin Fibers. Biopolymers 20: 1247-1260, 1981. 2. Arribas SM, Hinek A, and Gonzalez MC. Elastic fibres and vascular structure in hypertension. Pharmacol Ther 111: 771-791, 2006.
23
3. Bezie Y, Lacolley P, Laurent S, and Gabella G. Connection of smooth muscle cells to elastic lamellae in aorta of spontaneously hypertensive rats. Hypertension 32: 166-169, 1998. 4. Bezie Y, Lamaziere JMD, Laurent S, Challande P, Cunha RS, Bonnet J, and Lacolley P. Fibronectin expression and aortic wall elastic modulus in spontaneously hypertensive rats. Arterioscler Thromb Vasc Biol 18: 1027-1034, 1998. 5. Blacher J, Guerin AP, Pannier B, Marchais SJ, Safar ME, and London GM. Impact of aortic stiffness on survival in end-stage renal disease. Circulation 99: 2434-2439, 1999. 6. Boumaza S, Arribas SM, Osborne-Pellegrin M, McGrath JC, Laurent S, Lacolley P, and Challande P. Fenestrations of the carotid internal elastic lamina and structural adaptation in stroke-prone spontaneously hypertensive rats. Hypertension 37: 1101-1107, 2001. 7. Chamiot Clerc P, Renaud JF, Blacher J, Legrand M, Samuel JL, Levy BI, Sassard J, and Safar ME. Collagen I and III and mechanical properties of conduit arteries in rats with genetic hypertension. J Vasc Res 36: 139-146, 1999. 8. Chesler NC, Thompson-Figueroa J, and Millburne K. Measurements of mouse pulmonary artery biomechanics. J Biomech Eng-Trans ASME 126: 309-314, 2004. 9. Dobrin PB. Vascular mechanics. In: Handbook of Physiology, Section 2: The Cardiovascular System, edited by Chambers LS. Bethesda: American Physiological Society, 1983, p. 65-102. 10. Drexler ES, Quinn TP, Slifka AJ, McCowan CN, Bischoff JE, Wright JE, Ivy DD, and Shandas R. Comparison of mechanical behavior among the extrapulmonary arteries from rats. J Biomech 40: 812-819, 2007. 11. Durmowicz AG, Orton EC, and Stenmark KR. Progressive Loss of Vasodilator Responsive Component of Pulmonary-Hypertension in Neonatal Calves Exposed to 4,570 M. Am J Physiol 265: H2175-H2183, 1993. 12. Dyer K, Lanning C, Das B, Lee PF, Ivy DD, Valdes-Cruz L, and Shandas R. Noninvasive Doppler tissue measurement of pulmonary artery compliance in children with pulmonary hypertension. J Am Soc Echocardiogr 19: 403-412, 2006. 13. Et-Taouil K, Safar M, and Plante GE. Mechanisms and consequences of large artery rigidity. Can J Physiol Pharmacol 81: 205-211, 2003. 14. Fagan KA, Oka M, Bauer NR, Gebb SA, Ivy DD, Morris KG, and McMurtry IF. 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-L664, 2004. 15. Gundiah N, Ratcliffe MB, and Pruitt LA. Determination of strain energy function for arterial elastin: Experiments using histology and mechanical tests. J Biomech 40: 586-594, 2007. 16. Huang W, Delgado-West D, Wu JT, and Fung YC. Tissue remodeling of rat pulmonary artery in hypoxic breathing. II. Course of change of mechanical properties. Ann Biomed Eng 29: 552-562, 2001. 17. Humbert M, Morrell NW, Archer SL, Stenmark KR, MacLean MR, Lang IM, Christman BW, Weir EK, Eickelberg O, Voelkel NF, and Rabinovitch M. Cellular and molecular pathobiology of pulmonary arterial hypertension. J Am Coll Cardiol 43: 13S-24S, 2004. 18. Hunter KS, Lee PF, Lanning CJ, Ivy DD, Kirby KS, Claussen LR, Chan KC, and Shandas R. Pulmonary vascular input impedance is a combined measure of pulmonary vascular resistance and stiffness and predicts clinical outcomes better than pulmonary vascular resistance alone in pediatric patients with pulmonary hypertension. Am Heart J 155: 166-174, 2008.
24
19. Hyvelin JM, Howell K, Nichol A, Costello CM, Preston RJ, and McLoughlin P. Inhibition of rho-kinase attenuates hypoxia-induced angiogenesis in the pulmonary circulation. CircRes 97: 185-191, 2005. 20. Intengan HD and Schiffrin EL. Structure and mechanical properties of resistance arteries in hypertension - Role of adhesion molecules and extracellular matrix determinants. Hypertension 36: 312-318, 2000. 21. Intengan HD and Schiffrin EL. Vascular remodeling in hypertension: roles of apoptosis, inflammation, and fibrosis. Hypertension 38: 581-587, 2001. 22. Intengan HD, Thibault G, Li JS, and Schiffrin EL. Resistance artery mechanics, structure, and extracellular components in spontaneously hypertensive rats - Effects of angiotensin receptor antagonism and converting enzyme inhibition. Circulation 100: 2267-2275, 1999. 23. Jacob MP. Extracellular matrix remodeling and matrix metalloproteinases in the vascular wall during aging and in pathological conditions. Biomed Pharmacother 57: 195-202, 2003. 24. Jacob MP, Badier-Commander C, Fontaine V, Benazzoug Y, Feldman L, and Michel JB. Extracellular matrix remodeling in the vascular wall. Pathol Biol 49: 326-332, 2001. 25. Jacob MP and Ladislas R. Isolation, characterization and biochemical properties of elastin. In: Elastin and Elastases, edited by Ladislas R and Hornebeck W: CRC Press Inc., 1989, p. 45-69. 26. Kobs RW and Chesler NC. The mechanobiology of pulmonary vascular remodeling in the congenital absence of eNOS. Biomech Model Mechanobiol 5: 217-225, 2006. 27. Kobs RW, Muvarak NE, Eickhoff JC, and Chesler NC. Linked mechanical and biological aspects of remodeling in mouse pulmonary arteries with hypoxia-induced hypertension. Am J Physiol-Heart Circul Physiol 288: H1209-H1217, 2005. 28. Laurent S, Boutouyrie P, Asmar R, Gautier I, Laloux B, Guize L, Ducimetiere P, and Benetos A. Aortic stiffness is an independent predictor of all-cause and cardiovascular mortality in hypertensive patients. Hypertension 37: 1236-1241, 2001. 29. London GM, Blacher J, Pannier B, Guerin AP, Marchais SJ, and Safar ME. Arterial wave reflections and survival in end-stage renal failure. Hypertension 38: 434-438, 2001. 30. Lu Q, Ganesan K, Simionescu DT, and Vyavahare NR. Novel porous aortic elastin and collagen scaffolds for tissue engineering. Biomaterials 25: 5227-5237, 2004. 31. Mahapatra S, Nishimura RA, Jja PS, Cha S, and McGoon MD. Relationship of pulmonary arterial capacitance and mortality in idiopathic pulmonary arterial hypertension. J Am Coll Cardiol 47: 799-803, 2006. 32. Mahmud A and Feely J. Arterial stiffness and the renin-angiotensin-aldosterone system. J Renin Angiotensin Aldosterone Syst 5: 102-108, 2004. 33. Maruyama K, Ye CL, Woo M, Venkatacharya H, Lines LD, Silver MM, and Rabinovitch M. Chronic Hypoxic Pulmonary-Hypertension in Rats and Increased Elastolytic Activity. Am J Physiol 261: H1716-H1726, 1991. 34. Nagaoka T, Fagan KA, Gebb SA, Morris KG, Suzuki T, Shimokawa H, McMurtry IF, and Oka M. Inhaled rho kinase inhibitors are potent and selective vasodilators in rat pulmonary hypertension. Am J Respir Crit Care Med 171: 494-499, 2005. 35. Olsen MH, Christensen MK, Wachtell K, Tuxen C, Fossum E, Bang LE, Wiinberg N, Devereux RB, Kjeldsen SE, Hildebrandt P, Dige-Petersen H, Rokkedal J, and Ibsen H.
25
Markers of collagen synthesis is related to blood pressure and vascular hypertrophy: a LIFE substudy. J Hum Hypertens 19: 301-307, 2005. 36. Roach MR and Burton AC. The reason for the shape of the distensibility curves of arteries. Can J Biochem Physiol 35: 681-690, 1957. 37. Safar ME, Levy BI, and Struijker-Boudier H. Current perspectives on arterial stiffness and pulse pressure in hypertension and cardiovascular diseases. Circulation 107: 2864-2869, 2003. 38. Shadwick RE. Mechanical design in arteries. J Exp Biol 202: 3305-3313, 1999. 39. Sokolis DP, Boudoulas H, and Karayannacos PE. Assessment of the aortic stress-strain relation in uniaxial tension. J Biomech 35: 1213-1223, 2002. 40. Stenmark KR, Fagan KA, and Frid MG. Hypoxia-induced pulmonary vascular remodeling - Cellular and molecular mechanisms. CircRes 99: 675-691, 2006. 41. Stenmark KR and McMurtry IF. Vascular remodeling versus vasoconstriction in chronic hypoxic pulmonary hypertension - A time for reappraisal? CircRes 97: 95-98, 2005. 42. Van Gorp AW, Schenau DSV, Hoeks APG, Boudier H, De Mey JGR, and Reneman RS. In spontaneously hypertensive rats alterations in aortic wall properties precede development of hypertension. Am J Physiol-Heart Circul Physiol 278: H1241-H1247, 2000. 43. Weinberg C, Hertzberg J, Valdes-Cruz LM, and Shandas R. Extraction of pulmonary vascular compliance, PVR and RV work from single-pressure and Doppler flow measurements in children with pulmonary hypertension -- a new method for evaluating reactivity: In vitro and clinical studies. Circulation 110: 2609-2617, 2004. 44. Wohrley JD, Frid MG, Moiseeva EP, Orton EC, Belknap JK, and Stenmark KR. Hypoxia Selectively Induces Proliferation in a Specific Subpopulation of Smooth-Muscle Cells in the Bovine Neonatal Pulmonary Arterial Media. J Clin Invest 96: 273-281, 1995. 45. Wuyts FL, Vanhuyse VJ, Langewouters GJ, Decraemer WF, Raman ER, and Buyle S. Elastic properties of human aortas in relation to age and atherosclerosis: a structural model, 1995. 46. Zaidi SHE, You XM, Ciura S, Husain M, and Rabinovitch M. Overexpression of the serine elastase inhibitor elafin protects transgenic mice from hypoxic pulmonary hypertension. Circulation 105: 516-521, 2002. 47. Zhang Y, Dunn ML, Hunter KS, Lanning C, Ivy DD, Claussen L, Chen SJ, and Shandas R. Application of a microstructural constitutive model of the pulmonary artery to patient-specific studies: validation and effect of orthotropy. J Biomech Eng 129: 193-201, 2007. 48. Zhang YH, Dunn ML, Drexler ES, McCowan CN, Slifka AJ, Ivy DD, and Shandas R. A microstructural hyperelastic model of pulmonary arteries under normo- and hypertensive conditions. Ann Biomed Eng 33: 1042-1052, 2005. 49. Zulliger MA, Fridez P, Hayashi K, and Stergiopulos N. A strain energy function for arteries accounting for wall composition and structure. J Biomech 37: 989-1000, 2004.
26
Figure 1: Thickness measurements, tissue dissection and biopsy locations (typical). Internal Diameter (ID)
Figure 2: Detail of material testing system used to generate stress-strain data for arterial tissue samples.
Figure 3: Typical loading / unloading curves for fresh and elastin tissue tests.
Figure 4: Left: typical stress-strain behavior of fresh and elastin tissue, εtrans is the strain of transition from
the elastin-dominant region (A) to the transitional region (B) associated with increasing collagen engagement.
Right: typical curvature plot of fresh tissue.
Figure 5: Comparison of average thickness values and elastin area fractions between control and hypoxic
populations. (* P<0.05)
Figure 6: Comparison of mean values for artery stiffness and modulus of the RPA, LPA and MPA for control
and hypoxic populations. (* P<0.05)
Figure 7: Average control and hypertensive tissue stiffness at systolic and diastolic pressures. Comparative
values presented in table 1.
Figure 8: Comparison of mean values for elastin stiffness and modulus for the RPA, LPA and MPA for
control and hypoxic populations. (* P < 0.05)
Figure 9: Mean pressure-strain data for control and hypertensive tissues. Shaded regions indicate the
predicted physiologic conditions for control (A) and hypertensive (B) tissues.
Table 1: Average change in stiffness for control and PAH tissues at diastolic and systolic pressure and
average load carrying capacity of elastin. Comparative values based on the data presented in figure 7. ΦDias
27
(Sys), Cont to PAH: average increase in stiffness from control to PAH tissues measured at diastole (systole). ΦCont
(PAH), Dias to Sys: average increase in control (PAH) tissue stiffness from diastole to systole. %Fn Dias (Sys), Cont (PAH):
average percent load carrying capacity of control (PAH) tissue measured at diastole (systole). († P < 0.05)
ID-1
ID-2
Circumferential
MC3
ML3
MC2
ML2
MC1M
L1
Spare
Tissue anomaly (avoided)
Sec
tioni
ng P
lane
Thickness Measurement 4-Ortho. ea. side (8 total)
Axial View
Transverse Iso. View Sectioning Diagram
Biopsy tissueMech. test samples
5N Load Cell
A
A
Section AAMTS Detail
Buffer Solution
Rec
ycle
Loo
p
Fluid Level
5N L
oad
Cel
l
Thumb Screw
TissueGrips
ArterialTissueSample
Environmental Chamber Wall
−20 0 20 40 60 80−100
0
100
200
300
400
Strain (%)
Load
(m
N)
Fresh Tissue Raw Data, Fn − Strain Typ.
Preconditioning
Conditioned
−50 0 50 100 150−20
0
20
40
60
80
100
120
Strain (%)
Load
(m
N)
Elastin Tissue Raw Data, Fn − Strain Typ.
0 20 40 600
50
100
150
200
Strain ε (%)
Str
ess
σ (k
Pa)
Stress vs. Strain (Typ.)
Diastolic Stress
Systolic Stress
A B
σfresh
σelast
0 20 40 60 800
1
2
3
4
5x 10
−9 Strain vs. Curvature (Typ.)
Strain ε (%)
Cur
vatu
reκ
κAverage κ
PSS
εtrans
εL
εH
εPSS
H
κmax
κtrans
RPA LPA MPA0
1
2
3
4
5
6Average Thickness
Tissue Type
Thi
ckne
ss(m
m)
* *
*Control
Hypoxic
RPA LPA MPA0
10
20
30
40
50Average Area Fraction
Tissue Type
Are
a F
ract
ion
(%) * * *
RPA LPA MPA0
100
200
300
* * *
Artery Stiffness: Circumferential Direction
Tissue Type
Stif
fnes
sΦ
(m
m k
Pa)
RPA LPA MPA0
50
100
150
200
*
*
Artery Modulus: Circumferential Direction
Tissue Type
Mod
ulus
E (
kPa)
Control
Hypoxic
RPA LPA MPA0
1000
2000
3000
4000Average Artery Stiffness for Systolic and Diastolic Pressures
Tissue Type
Stif
fnes
sΦ
(m
m k
Pa)
RPA LPA MPA0
100
200
300
400Average Elastin Stiffness for Systolic and Diastolic Pressures
Tissue Type
Stif
fnes
sΦ
(m
m k
Pa)
Diastolic Control Diastolic Hypoxic Systolic Control Systolic Hypoxic
RPA LPA MPA0
50
100
150
200
* *
*
Elastin Stiffness: Circumferential Direction
Tissue Type
Stif
fnes
sΦ
(m
m k
Pa)
RPA LPA MPA0
50
100
150
200
* *
Elastin Modulus: Circumferential Direction
Tissue Type
Mod
ulus
E (
kPa)
Control
Hypoxic
RPA LPA MPA Average RPA LPA MPA Average
Dias, Cont to PAH 327%† 274%† 279%† 293%† 151%† 243%† 124%† 173%†
Sys, Cont to PAH 584%† 512%† 435%† 510%† 102%†186% 81%† 123%†
Cont, Dias to Sys 151%† 125%†158% 145%†
41% 41% 36% 39%
PAH, Dias to Sys 303%† 268%† 265%† 278%†13% 18% 10% 14%
RPA LPA MPA Average%Fn Dias, Cont 50% 46% 87% 61%%Fn Dias, PAH 45% 43% 56% 48%%Fn Sys, Cont 45% 36% 63% 48%%Fn Sys, PAH 30% 31% 35% 32%
Table 1. Physiologic stiffness comparison Fr
esh
Tiss
ue
Ela
stin
Tis
sue
Percent load carrying capacity of elastin
top related