reversible permeabilization using high-intensity femtosecond laser pulses: applications to...
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Reversible Permeabilization UsingHigh-Intensity Femtosecond Laser Pulses:Applications to Biopreservation
Vikram Kohli,1 Jason P. Acker,2,3 Abdulhakem Y. Elezzabi1
1Ultrafast Photonics and Nano-Optics Laboratory, Department of Electrical andComputer Engineering, University of Alberta, Edmonton, Alberta, Canada2Canadian Blood Services, Research and Development, 8249-114 Street, 3rd Floor,Edmonton, Alberta, Canada T6G 2R8; telephone: þ780-702-8629; fax: þ780-702-2501;e-mail: [email protected] of LaboratoryMedicine and Pathology, University of Alberta, Edmonton,Alberta, Canada
Received 8 May 2005; accepted 23 June 2005
Published online 27 September 2005 in Wiley InterScience (www.interscience.wiley.com). DOI: 10.1002/bit.20689
Abstract: Non-invasive manipulation of live cells isimportant for cell-based therapeutics. Herein we reporton the uniqueness of using high-intensity femtosecondlaser pulses for reversibly permeabilizing mammaliancells for biopreservation applications. When mammaliancells were suspended in a impermeable hyperosmo-tic cryoprotectant sucrose solution, femtosecond laserpulses were used to transiently permeabilize cells forcytoplasmic solute uptake. The kinetics of cells exposed to0.2, 0.3, 0.4, and 0.5 M sucrose, following permeabiliza-tion, were measured using video microscopy, and post-permeabilization survival was determined by a dualfluorescence membrane integrity assay. Using appropri-ate laserparameters,weobserved thehighest cell survivalfor 0.2 M sucrose solution (>90%), with a progressivedecline in cell survival towards higher concentrations.Using diffusion equations describing the transport ofsolutes, the intracellular osmolarity at the inner surfaceof the membrane (x ¼10 nm) and to a diffusive length ofx ¼10 mm was estimated, and a high loading efficiency(>98% for x ¼10 nm and >70% for x ¼10 mm) wascalculated for cells suspended in 0.2 M sucrose. This isthe first report of using femtosecond laser pulses forpermeabilizing cells in the presenceof cryoprotectants forbiopreservation applications. � 2005 Wiley Periodicals, Inc.
Keywords: femotsecond; ultrashort laser pulses; per-meabilization; cryoprotectant; sugars; biopreservation;cryobiology; cryopreservation
INTRODUCTION
With the recent advancements in tissue engineering, cell
transplantation, and genetic technologies, living cells as a
therapeutic tool for clinical care have receivedwide attention
(Acker et al., 2004). These emerging technologies depend on
the characteristics of living cells, and thus maintaining and
preserving the biological function of cell-based therapeutics
remains one of the most important challenges facing
reparative medicine (Acker, 2005).
The goal of biopreservation is to protect the integrity
and functionality of living cells, tissues, and organs, which
has resulted in the development of techniques that can
achieve biological stability and ensure a viable state follow-
ing ex vivo storage (Acker, 2005; Acker et al., 2004).
Cryopreservation has been the traditional approach used for
long-term preservation. In this process, cells are frozen
to ultra low temperatures (i.e., �80 to �1968C) where
molecular motion is suppressed and biochemical and meta-
bolic reactions are arrested. Achieving cell preservation at
cryogenic temperatures requires a proper balance between
the cooling rates, thawing rates, and cryoprotectant concen-
tration (Diller, 1975; Fahy et al., 1984; Lovelock, 1953;
Mazur, 1984).
Efforts to improve post-thaw cell survival have focused
on the role of cryoprotectants in stabilizing and protecting
cells from lethal injury. Low-molecular weight permeating
cryoprotectants such as methanol, ethylene glycol, glycerol,
and dimethyl sulfoxide have been routinely used in cryo-
preservation studies (Lovelock, 1953; Palasz and Mapletoft,
1996). However, more recently, low concentrations of mem-
brane impermeable disaccharides (trehalose and sucrose),
have received wide attention (Acker, 2005; Acker et al.,
2004; Chen et al., 2001; Crowe et al., 2001; Fabbri
et al., 2001). The mechanism of sugar protection is an active
area of research that includes the role of the glassy state in
long-term stabilization (Buitink et al., 1998; Crowe et al.,
1998), the interaction of sugars with biological molecules
and supramolecular structures to afford stabilization (Crowe
et al., 1988) and the role that the unique physico-chemical
properties of sugars have during freezing and thawing
(Crowe et al., 2004). Regardless of the mechanism of action,
�2005 Wiley Periodicals, Inc.
Correspondence to: J.P. Acker
Contract grant sponsors: Canadian Blood Services (CBS); Natural
Sciences and Engineering Research Council of Canada (NSERC); Infor-
matics Circle of Research Excellence (iCORE); Canada Foundation for
Innovation (CFI)
the protective effect of cryoprotective sugars has been
demonstrated in a wide variety of biological systems (Acker
et al., 2003; Buchanan et al., 2004; Chen et al., 2001;
Crowe et al., 2001; Eroglu et al., 2000, 2002; Satpathy et al.,
2004).
Since non-reducing disaccharides are impermeable to the
lipid bilayer, several methods have been used for permeabi-
lizing cells for cytoplasmic sugar uptake. These include
microinjection, osmotic and thermal shock, genetic engi-
neering, electroporation, and the use of bacterial pore-
forming toxins (Acker et al., 2003; Buchanan et al., 2004;
Eroglu et al., 2000, 2002).While each method has significant
benefits, the tedious process of microinjection (Acker et al.,
2004) and the irreversible cell damage induced by electro-
poration (including membrane bleb formation, disruption of
biochemical pathways, DNA denaturation, and cell lysis
(Acker et al., 2004; Kinosita and Tsong, 1977; Tsong, 1991;
Vernhes et al., 1999; Weaver, 1993) have limited their use in
clinical applications. Genetic engineering and thermal and
osmotic shock have been shown to be effective at overcoming
the impermeability ofmammalianmembranes, but the extent
to which sugars are accumulated intracellularly may be
insufficient to confer protection (Acker et al., 2004).
Furthermore, bacterial a-toxins induce irreversible mem-
brane damage and may have potential cytotoxic and
immunogenic effects (Acker et al., 2003; Buitink et al.,
1998; Tsong, 1991; Thelestam, 1983). In order to achieve
high post-permeabilization and post-thaw survival rates, it is
important that the permeabilization tool be applicable to all
cell types without inducing deleterious effects.
Recently, the application of high-intensity ultrashort
(femtosecond) laser pulses has been shown to have important
implications for studying live cells (Koenig et al., 1999;
Kohli et al., 2005; Matsunaga et al., 2004). The lasers
contact-free and non-invasive nature allows for cells to be
manipulated in a precise and controlled fashion. Since
the pulse duration of femtosecond lasers is shorter than
the thermal diffusion time (picoseconds to nanoseconds),
thermal shock and mechanical damage is insignificant
(Kohli et al., 2005; Tirlapur and Koenig, 2002a,b; Niemz,
2002).
The purpose of this study was to evaluate the effective-
ness of using femtosecond laser pulses to reversibly
permeabilize mammalian cells. Our goal was to demon-
strate the generation of transient optical pores, and the
cytoplasmic uptake of cryoprotectant sugar. We evaluated
the kinetics of cells suspended in a hyperosmotic solution of
sucrose, and measured the volumetric change upon per-
meabilization. Using appropriate laser parameters, the
optimal cell survival rate as a function of cryoprotectant
concentration was determined. To ensure efficient post-
permeabilization cryoprotectant loading, the solute trans-
port equation for a porous membrane was used to estimate
the intracellular accumulation of sugar. To date, no report
has documented the applicability of using ultrashort laser
pulses for intracellular delivery of sugar for biopreservation
applications.
MATERIALS AND METHODS
Cell Culture
Madin-Darby Canine Kidney cells (MDCK; American Type
Culture Collection (ATCC) CCL-34) were cultured at 378Cin an atmosphere of 95% air plus 5% carbon dioxide in
supplemented medium consisting of minimum essential
media with Hanks salts, 16 mmol/L sodium bicarbonate,
2 mmol/L L-glutamine, and 10% fetal bovine serum (all
components from Hyclone Laboratories, Logan, UT). Cells
in exponential growth phase were harvested by exposure to a
0.25% trypsin–1 mM EDTA solution at 378C, washed twicewith supplemented medium, plated onto sterile, micropat-
terned glass coverslips (12mm2FisherBrand) and cultured at
378C for 12 h to allow the cells to attach.
Cell Micropatterning
A simplified cell micropatterning method (Chen et al., 1998)
using a polydimethylsiloxane (PDMS) elastomeric stamp to
create non-adhesive regions of agarose on glass substrate
allowed for precise control of cell geometry. Using micro-
patterned cells allowed for accurate retrospective analysis of
cell viability following laser permeabilization.
Photolithography
Four-inch silicon wafers were bathed in a piranha solution
consisting of sulphuric acid (J.T. Baker, Phillipsburg, NJ) and
hydrogen peroxide (J.T. Baker) in a 3-to-1 ratio for 15 min.
The wafers were rinsed in deionized water and dried using
nitrogen. A layer of hexamethyldisilazane (Arch Chemicals,
Norwalk, CT) was spin-coated onto the silicon wafers and
baked at 1508C for 10 min to improve photoresist adhesion.
A 10 mm layer of Microposit SJR 5740 positive photoresist
(Shipley,Marlborough,MA)was spin-coated onto thewafers
and baked at 1158C for 6min. For pattern transfer, the wafers
were exposed for 18 s to ultraviolet light at a constant
intensity of 18.1 mW/cm2. The pattern was transferred from
an acetate mask produced by high-resolution printing
(Advance Reproductions, North Andover, MA) and con-
sisted of a matrix of rectangles of dimensions 30� 30 mmwith a well separation of 60 mm.
Preparation of the PDMS Stamps
PDMS stamps were prepared by mixing prepolymer and a
curing agent in a 10:1 ratio by weight as indicated by the
manufacturer (Corning, NY). The polymerwas cured at 708Cfor 1 h in a vacuum, and was peeled off the wafers and used
for patterning of glass substrates.
Patterning of the Glass Coverslips With Agarose
PDMS stamps were placed pattern side down on glass
coverslips. A 0.6 g/100 mL low-melting point agarose
890 BIOTECHNOLOGY AND BIOENGINEERING, VOL. 92, NO. 7, DECEMBER 30, 2005
(Invitrogen Corporation, Carlsbad, CA)/40% ethanol (VWR
Can Lab, Brampton, Ont., Canada) solution was prepared
and injected through the channels of the micropatterns. The
coverslips were placed in a vacuum chamber for 18 h to dry.
Following drying, the stamps were peeled off, leaving
patterned agarose on the glass substrate.
Cell Viability Assessment
A dual fluorescent staining technique was used for quanti-
tative assessment of the integrity of the cell plasma
membrane (Yang et al., 1998). SYTO 13TM (Molecular
Probes, Eugene, OR) and ethidium bromide (EB; Sigma
Chemical Company, Mississauga, Ont., Canada) were used
to differentially stain the cells. SYTO readily permeates
intact cells and fluorescently labels both RNA and DNA
green. EB has been shown to penetrate only cells with
damaged membranes and forms a fluorescent red complex
with nuclear DNA (Edidin, 1970). The SYTO/EB assay for
membrane integrity has been previously shown to correlate
well with other assessment techniques for cell viability (Yang
et al., 1998). Percent survival based on membrane integrity
was calculated as the number of SYTO positive cells over the
total number of cells.
Cell Volume Measurements
The volumetric response of micropatterned MDCK cells in a
hypertonic solution of sucrose was used to assess solvent
mass transport. The estimated volumetric response of the
cells to a transient pore was determined by measuring the
diameter of the cell, along both the x- and y-axis, as a function
of time using image analysis software (ImageJ, National
Institutes of Health). The measurements were averaged
to minimize errors in the approximation of the volume.
Assuming a spherical geometry, cell volumes were then
calculated.
Intracellular Solute Delivery Estimation
A modified diffusion equation for solute transport through a
porous membrane was used to estimate the intracellular
accumulation of cryoprotectant sugar for cells in 0.2, 0.3, and
0.5 M sucrose suspensions. From Fick’s law of diffusion, the
solute flux rate of sucrose in water is (Finkelstein, 1987)
Fsw ¼ Dsw
DCs
Dxð1Þ
where Fsw is the flux transport rate of the solutes in water,
Dsw is the diffusion coefficient of the solutes in water, DCs is
the solute concentration difference across the cell mem-
brane, and Dx is the distance defined by DCs. Since sucrose
is impermeable to the plasma membrane, the permeabiliza-
tion of the cell by femtosecond laser pulses provides the
transport mechanism for cytoplasmic sugar uptake. Equa-
tion (1) can then be modified to represent the solute
transport flux through a pore (Finkelstein, 1987)
Fsw ¼ nA
LDsw
DCs
Dxð2Þ
where A is the area of the pore, L is the length of the pore,
and n is the number of pores. Absorbing A, L, n, Dx, and Dsw
into a constant, denoted as D0, noting from the continuity
equation that the one-dimensional time rate of change in
solute concentration is (Smits, 2000)
@Csðx; tÞ@t
¼ *r � Fsw ð3Þ
and substituting Equation (2) into Equation (3), then solving
for Cs (x, t) subject to initial conditions, Cs (0, t)¼C0 and Cs
(1, t)¼ 0
Csðx; tÞ ¼ C0erfcx
2ffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiffiðnDswAt=LDxÞ
p !
ð4Þ
yields a modified equation for Fick’s 2nd law of diffusion
describing solute flux through a membrane pore. In
Equation [4] Cs (x, t) is the concentration of solutes, C0 is
the initial concentration of solutes, t is time, x is the distance
over which Cs (x, t) is computed, and erfc is the
complementary error function. The length of the pore is
a constant equal to the thickness of the cell membrane
(L¼ 10 nm), and A was taken to be the area of the pore
generated by the focused femtosecond laser pulses, where
the diameter was equal to the laser spot size. Cs (x, t) was
calculated as a function of distance along the pore, with C0
equal to the extracellular osmolarity, and t was set to the
time required for the cell to reach equilibrium volume post-
permeabilization. The diffusion coefficient of sucrose in
water was determined using Einstein’s fluctuation–dissipa-
tion formula, where a single sucrose molecule was modeled
as a sphere with a defined diameter. To estimate the diameter
of a sucrose molecule, bond lengths were added along the
long axis yielding a calculated diameter of 1.6 nm.
Laser Microscope Setup
Optical permeabilization ofmicropatternedMDCKcells was
achieved using a modelocked titanium sapphire laser
oscillator, producing sub-10 femtosecond laser pulses, with
a center wavelength of 800 nm and a repetition rate of
80 MHz. The laser pulses were coupled to a modified optical
microscope and directed towards the biological sample, as
shown in Figure 1. To focus the femtosecond pulses, a 0.95
high numerical aperture microscope objective was used,
producing a spot size of <1 mm. Using an average delivered
power of 270–410mW, 3–5 nJ pulses were generated within
the focal volume and dynamically gated using a mechanical
shutter.MicropatternedMDCKcells were placed on an x–y–
z translation stage for precise sample movement, and the
stage was temperature controlled to 48C. Optical permeabi-
lization was viewed with a charge coupled device mounted
on the modified optical microscope and captured using
commercial video software.
KOHLI ET AL.: REVERSIBLE PERMEABILIZATION USING FEMTOSECOND LASERS 891
Statistical Analysis
Unless otherwise stated, all uncertainty calculations were
determined using the error propagation formula. Assuming
that fluctuations in the function were uncorrelated, all
covariant terms were set to zero.
RESULTS
Laser Induced Optical Poration
Before permeabilizing mammalian cells in the presence of
impermeable cryoprotectants, we first assessed the feasi-
bility of using a femtosecond laser to create optical pores
in micropatterned cells. Using an average laser power of
410 mWand a gated shutter time of<10 ms, sub-10 fs laser
pulses were coupled and focused by a 0.95 high numerical
aperture microscope objective. A focal spot of <1 mm in
diameter was generated at the focal plane of the membrane,
with a total energy absorption of 4 mJ over the gated
femtosecond pulse train. To evaluate the presence of a pore,
the dual fluorescence membrane integrity assay SYTO/EB
was used. The mammalian cells were stained �10–20 min
post-laser exposure. Figure 2a depicts bright field images
of micropatterned cells before laser exposure, where the
arrows indicate cells that have been selectively targeted for
permeabilization. In Figure 2b, a fluorescence image after
permeabilization is shown. Micropatterned MDCK cells
exposed to femtosecond laser pulses were positive for
EB staining, indicating a damaged permeable plasma
membrane.
Intracellular Delivery ofSucrose Using Optical Pores
To determine whether optical pores are sufficiently large
and open for a duration that permits sucrose diffusion, the
volumetric response of MDCK cells suspended in 1.0 M
sucrose was evaluated. Figure 3a depicts the shrunken
appearance of three MDCK cells suspended in a hypertonic
solution of 1.0M sucrose. In Figure 3a, a single cell has been
selected for permeablization, and the focused femtosecond
laser spot is shown. When the ultrashort (femtosecond)
pulses were focused to a spot size of <1 mm, a transient
optical pore was created in the individual cell, exposing the
cytoplasm to the extracellular environment. Once exposed,
Figure 1. Experimental setup. A Kerr lens modelocked titanium sapphire laser oscillator, producing sub-10 femtosecond laser pulses, with a center
wavelength of 800 nm and a repetition rate of 80MHzwas directed towards a 0.95 high numerical aperturemicroscope objective. The ultrashort (femtosecond)
pulses were focused onto the cell with a focal spot of <1 mm. The cells were placed on a temperature-controlled stage cooled to 48C. To visualize reversiblepermeabilization, the cells were illuminated from beneath with white light, and imaged using a charge coupled device (CCD) and processed by commercial
video capture software.
892 BIOTECHNOLOGY AND BIOENGINEERING, VOL. 92, NO. 7, DECEMBER 30, 2005
an increase in cellular volume was observed, Figure 3b, with
the increase occurring only in the targeted cell. To deter-
mine the hypertonic to equilibrium volumetric response of
micropatterned MDCK cells, the volume was calculated
(presuming a spherically shaped cell) before and after
permeabilization. In hypertonic conditions, an equilibrium
V/Vequil¼ 0.578� 0.085 was measured versus V/Vequil¼1.000� 0.055 at equilibrium volume post-permeabilization.
Therefore, an approximate 60% change in volume was
observed when the cell was porated using femtosecond laser
pulses in the presence of 1.0 M sucrose.
The kinetics of MDCK cells suspended in various
hyperosmotic solutions of sucrose were also measured.
Using video microscopy, the change in volume of cells
porated with femtosecond laser pulses was measured as a
function of time. Before permeabilization, the initial equili-
brium cell volume in the solution was determined, and upon
poration, the return to equilibrium volume was measured.
Figure 4 depicts the kinetics of a single mammalian cell
suspended in a 0.2 M sucrose solution. All calculated values
for the volume were normalized to the post-permeabilized
equilibrium volume, as determined from direct measure-
ments. Similar volumetric response graphswere observed for
micropatterned MDCK cells suspended in 0.3 and 0.5 M
sucrose (data not shown). Cells suspended in 0.2 M sucrose
took less than 270 ms to return to equilibrium volume
following laser permeabilization.
Figures 5 and 6 illustrate the results of our laser perme-
abilization method for MDCK cells in a 0.2, 0.3, 0.4, and
0.5 M sucrose solution. The bright field image in Figure 5
represents live cells suspended in a 0.2 M hyperosmotic
sucrose solution pre-laser exposure, while the fluorescence
images depict cell viability 30–40 min post-exposure.
In Figure 5, a total of six cells were laser exposed (cell 5
detached from the well post-permeabilization), indicated by
the numbers 1–6 (fluorescence and bright field images for
0.3, 0.4, and 0.5 M not shown). The fluorescence images
in Figure 5 depict live MDCK cells, which have intact
membranes and optical pores that have completely sealed.
This is evident from the absence of EB diffusion, which
stains the cells red-orange for membranes that have been
compromised.
Figure 2. Laser-induced optical pore. a: Represents a bright-field image of live micropatternedMDCK cells. Using an average laser power of 410mW, and a
gated shutter time of<10ms, sub-10 fs laser pulses were coupled and focused by a 0.95 high numerical aperturemicroscope objective to generate a sub-micron
focal spot. The arrows in (a) represent cells selected for laser permeabilization. Approximately 10–20 min post-permeabilization the cells were stained with
SYTO/EB to evaluate the presence of a pore. b: The fluorescent image depicts the cytoplasmic uptake of EB for laser-permeabilized cells, as represented by the
arrows. Scale bar in (a) is 40 mm; scale bar in (b) is 100 mm. [Color figure can be seen in the online version of this article, available at www.
interscience.wiley.com.]
Figure 3. The response of a micropatternedMDCK cell suspended in 1.0 M sucrose when permeabilized by femtosecond laser pulses. a: MDCK cell before
permeabilization. The arrow depicts the focused femtosecond laser spot. Only one cell was chosen for permeabilization, demonstrating the precision of the
process. b:MDCK cell after permeabilization. The cell has increased in cellular size towards equilibrium volume. The arrow in (b) illustrates the permeabilized
cell. Scale bar in (a) and (b) is 40 mm.
KOHLI ET AL.: REVERSIBLE PERMEABILIZATION USING FEMTOSECOND LASERS 893
When the micropatterned MDCK cells were suspen-
ded in an increasingly hypertonic solution (0.3 M; n¼ 7,
0.4 M; n¼ 15, 0.5 M; n¼ 8), post-permeabilized cells
exhibited an increase in membrane damage. Figure 6
illustrates cell survival as a function of sucrose concentra-
tion under constant laser power and energy absorption.
A post-laser exposure survival rate of 91.5� 8% was
achieved using an extracellular sucrose concentration of
0.2 M.
Percentage Intracellular Uptake
Using Equations (2–4), an estimate of the intracellular solute
delivery was calculated, and is presented in Table I. From
Equation (4), with n¼ 1, the solute concentration, Cs (x, t),
was computed for each cryoprotectant sucrose solution,
where t for each solutionwas determined from thevolumetric
response plots at equilibrium volume post-permeabilization.
Figure 7 depicts the change in solute concentration as a
Figure 4. Volumetric response of a micropatternedMDCK cell in a 0.2 M
cryoprotectant sucrose solution. Initially the cell is in a shrunken state.
Upon laser permeabilization, the cell quickly swells to equilibrium volume.
The value ofVequil was taken to be the equilibrium volume asmeasured using
ImageJ.
Figure 5. Laser permeabilized micropatterned MDCK cells suspended in a 0.2 M cryoprotectant sucrose solution. a: Represents bright field images of
micropatterned cells where the numbers indicate cells selected for permeabilization. All cells were treatedwith an average laser power of 270mWusing a gated
shutter time of<10 ms with a total energy absorption of<2 mJ. After treatment, a change in cell volume from hypertonic equilibrium volume to equilibrium
volumewas observed. b: The cells were stained with SYTO/EB approximately 30–40 min post-laser exposure. The absence of EB diffusion indicates that the
cells were permeabilizedwith reversible pores. Cell 5 detached from themicropatternedwell post-permeabilization. Scale bar in (a) is 40 mm; scale bar in (b) is
100 mm. [Color figure can be seen in the online version of this article, available at www.interscience.wiley.com.]
Figure 6. Cell survival post-laser exposure as a function of the
extracellular solute concentration. A progressive decline in cell survival
with increasing solute concentration is observed. Highest cell viability was
obtained forMDCKcells suspended in 0.2Msucrose.No cells survived post-
laser exposure in a 0.5 M sucrose suspension.
894 BIOTECHNOLOGY AND BIOENGINEERING, VOL. 92, NO. 7, DECEMBER 30, 2005
function of distance through the pore for cells in a 0.2 M
sucrose suspension. Since the average thickness of a cell
membrane is 10 nm, diffusion of solutes to a distance of
x¼ 10 nm would constitute intracellular sucrose accumula-
tion. Cs (10 nm, tequil) from Figure 7 for cells suspended
in 0.2 M sucrose was estimated to be Cs (10 nm, tequil)¼0.199 M with a loading efficiency of 99% to a distance just
inside the plasma membrane. Similar diffusion profiles were
obtained for 0.3 and 0.5 M sucrose. Cs (10 nm, tequil) for
0.3 and 0.5 Mwere estimated to be 0.299 and 0.499Mwith a
loading efficiency of 99% for each osmolarity. The inset in
Figure 7 represents the diffusion profile plotted to large
diffusion lengths. From the inset, the sucrose concentration at
a distance of x¼ 10 mm within the cell was estimated to be
Cs (10 mm, tequil)¼ 0.145, 0.198, and 0.330 M for cells
suspended in 0.2, 0.3, and 0.5 M sucrose.
DISCUSSION
Induced Transient Pores byFemtosecond Laser Pulses
Intracellular sugars are increasingly being used in the
development of effective technologies for the preservation
of cells and tissues used in reparative medicine. To assess the
usefulness of using femtosecond laser pulses for biopreser-
vation applications, we first evaluated their ability to create
transient pores for the selective uptake of cryoprotectants. As
shown in Figure 2, the creation of optical pores allows for
intracellular solute uptake.When the cells were suspended in
SYTO/EB, the localized pore facilitated the diffusion of EB
into the cytoplasm of the cell. Since the molecular weight of
EB (394 g/mol) and sucrose (342 g/mol) are comparable, the
diffusion of EB suggests that the optical pore should be large
enough to allow the cytoplasmic uptake of cryoprotective
disaccharides. In Figure 2b, the red labeled complex stains
for membrane integrity, indicating that the porated cells are
compromised. Proper adjustments to pulse energy, pulse
duration, and energy absorption can precisely control both
the size and dynamics of the pore. This makes femtosecond
lasers an ideal tool for microscopic manipulation of unfixed
specimens.
Determination of the Optimal Laser Parameters
We observed that focused femtosecond laser pulses could
efficiently permeabilize living cells (Fig. 2). We have
determined through previous studies (unpublished data) that
as the energy absorption of the cell increases, necrotic
behavior also increases. In order to avoid irreparable cell
damage, gating the laser pulses with a mechanical shutter of
<10 ms in duration, a total laser energy absorption of<2 mJ
provides the optimal laser parameters for optical poration
while maintaining maximized post-permeabilization survi-
val rates. Cell survival was determined by SYTO/EB, and
while the dual assay is not an absolute measure of viability, it
has beenwidely used in characterizing cell death (Chen et al.,
2001). Therefore, for all subsequent experiments we used
SYTO/EB for measuring viability, and an average laser
power of 270 mW gated at <10 ms was chosen.
Table I. Calculated values for the intracellular accumulation of sucrose at a length of 10 nm and 10 mmwithin
the cell.
Constants
Initial concentration
(molecules/cm3) tequil (s) Cs (x, tequil) (M)
A¼ 0.785� 0.392 mm2 C0¼ 1.204E20 (0.2 M) tequil¼ 0.20 (0.2 M) x¼ 10 nm
T¼ 277 K C0¼ 1.806E20 (0.3 M) tequil¼ 0.13 (0.3 M) Cs¼ 0.199 (0.2 M)
L¼ 10 nm C0¼ 3.011E20 (0.5 M) tequil< 0.13 (0.5 M) Cs¼ 0.299 (0.3 M)
Dsw¼ 2.536E-6 cm2/s Chosen to be 0.13 Cs¼ 0.499 (0.5 M)
x¼ 10 mmCs¼ 0.145 (0.2 M)
Cs¼ 0.198 (0.3 M)
Cs¼ 0.330 (0.5 M)
Figure 7. Diffusion profile for a cell suspended in an extracellular
osmolarity of 0.2 M sucrose following permeabilizaton. Using the modified
diffusion equation for a porousmembrane, the diffusion of sucrose across the
porewas calculated as a function of pore length,with t equal to the time taken
for the cell to reach equilibrium volume. For a cell membrane thickness of
10 nm, the intracellular accumulation of sucrosewas estimated to be 0.199M
at the inner surface of the plasma membrane. The inset depicts the diffusion
profile for large diffusion lengths. The concentration at a length of 10 mmwithin the cell was estimated to be 0.145, 0.198, and 0.330M for cells in 0.2,
0.3, and 0.5 M sucrose suspensions.
KOHLI ET AL.: REVERSIBLE PERMEABILIZATION USING FEMTOSECOND LASERS 895
The Kinetics of Optical Pores
Despite the similar molecular weights of EB and sucrose, we
measured the volumetric response of mammalian cells
suspended in varying hyperosmotic solutions of sucrose as
a means to more directly monitor pore dynamics and sugar
uptake. If the transient pore provides the mechanism for
sucrose diffusion, then the kinetics should reveal a cell that
has increased in cellular volume. This method for verifying
the uptake of sucrose, based on the volumetric response, has
been employed and well characterized by Eroglu and Russo
et al. (Eroglu et al., 2000; Russo et al., 1997). Russo showed
that the volumetric response of fibroblast cells permeabilized
by a bacterial a-toxin in the presence of a hypertonic sucrosesolution was an increase in cell size towards equilibrium
volume, resulting from the intracellular uptake of sucrose
(Russo et al., 1997). Figure 4 depicts a cellular increase,
where the volume change as a function of time for a cell
suspended in 0.2 M sucrose has been plotted. Upon poration,
the cell quickly swells from hypertonic volume to equili-
brium volume. Similar volumetric plots were found for
mammalian cells in 0.3 and 0.5 M sucrose (data not shown).
The upward trend depicted in Figure 4, towards an increased
cell volume, agrees well with the volumetric response plots
found by Russo et al., and is consistent with the observed
change in cell volume due to intracellular sugar uptake
(Russo et al., 1997).
Viability of Micropatterned MDCK CellsPermeabilized by Femtosecond Laser Pulses
When live mammalian cells were exposed to high-intensity
femtosecond laser pulses, the laser was shown to be an
efficient tool for the introduction of cryoprotectants. Figure 6
depicts the survival rate as a function of increasing molar
concentrations of sucrose. As the trend suggests, cell survival
is maximized at 0.2 M (91.5� 8%) and progressively
decreases with higher sucrose concentrations. These results
are consistent with pre-freeze mammalian cells porated
using a-hemolysin by Eroglu et al., where the survival of
permeabilized fibroblast cells decreased from 98.1� 6.4 to
84.1� 3.3% using 0.2 and 0.4 M trehalose (Eroglu et al.,
2000). We found that with 0.5 M sucrose, a 0% survival rate
was observed, while a 45% increase in survival occurred
when themolar concentration was changed from 0.4 to 0.3M
sucrose. Using a 0.3 and 0.4M sucrose solution, we observed
a pre-freeze survival of 75� 5 and 30� 10%. We hypothe-
size that the progressive decline in cell survival with
increasingly hyperosmotic solutions may be due to transient
pore widening (Muldrew, 2003) leading to osmotic poration
injury (Muldrew and McGann, 1994).
Osmotic Poration Injury
Muldrew and McGann (1994) proposed an osmotic rupture
hypothesis, in which osmotically driven water induced
osmotic stress and caused rupturing of the plasmamembrane.
The stress resulted from the sudden movement of water in
response to an increasing concentration of extracellular
solutes when mammalian cells were cooled to sub-zero
temperatures. A mathematical model was developed, where
the frictional force on the membrane was converted to a
pressure term describing the pressure exerted on the
membrane resulting from water efflux (Muldrew and
McGann, 1994). Muldrew and McGann showed that the
frictional force was proportional to the water flux, Fw, and
that the pressure induced on themembrane increasedwithFw
(Muldrew andMcGann, 1994). The uniform pressure exerted
on the membrane caused a rupture, leading to a spontaneous
breakdown in the symmetry of the membrane’s tensile
strength (Muldrew and McGann, 1994).
When cells are placed in a solution containing a high
concentration of impermeant solutes, water moves out of the
cell along its concentration gradient towards a lower
chemical potential. Subsequently, the cell dehydrates until
the intracellular and extracellular osmolalities are equal.
Varying the extracellular osmolarity from a lower concentra-
tion to a higher concentration results in an increase in the
water flux across the cell membrane, as larger volumes of
water are required to dilute higher impermeant solute
concentrations. When the cells are permeabilized, water
quickly diffuses into the cell, driven by the changing solute
gradient. The passive diffusion of the solutes towards a lower
chemical potential drags the water molecules towards the
inside of the cell, and a new equilibrium cell volume is
obtained.We believe, by invoking theMuldrew andMcGann
hypothesis, that the decrease in cell survival with increasing
solute concentration can be explained by pore widening that
occurs when the trans-membrane osmotic gradient increases.
In our experiment, when femtosecond pulses were focused
onto the cell membrane, a pore of <1 mm in diameter was
created. The pore provided the transport mechanism for the
intracellular accumulation of sucrose as well as water. Since
Muldrew andMcGann showed that frictional forces arise due
to water movement across the cell membrane, we expected
similar forces to develop along the length of the transient
pore. Relating the force to pressure, the osmotically active
water diffusing through the pore would place pressure on the
pore, resulting in its widening. The amount of induced
pressure would depend on Fw, and Fw would increase with
extracellular osmolarity. We expected the pressure to be
increased by our permeabilization process, as the predomi-
nant mode of water transport would be through the pore (the
least resistive path to water movement). The uniform
pressure would be confined to the area of the pore, and not
distributed over the entire membrane, as in the case of
Muldrew and McGann (1994). The typical transit time for
water influx or efflux through a cell membrane is seconds to
minutes, where the rate of water movement is governed by
the membrane hydraulic conductivity, Lp, and the osmotic
water permeability, Pf (Elmoazzen, 2000). From Figure 4,
we notice that a cell in 0.2 M sucrose suspension reached
equilibrium volume in less than 270 ms at a temperature of
48C. Passive diffusion of water through the membrane,
896 BIOTECHNOLOGY AND BIOENGINEERING, VOL. 92, NO. 7, DECEMBER 30, 2005
facilitated by an osmotic gradient, cannot account for
the observed cellular volume increase within the defined
temperature and time. For the volume to increase towards
equilibrium in less than 270 ms would require water to be
predominately transported through the transient pore. Since
the uniformpressurewould be confined to the area of the pore,
we would expect pore widening to occur. The degree of
wideningwould increasewith extracellular osmolarity due to
the dependency of Fw on concentration. The effect of
an increasing pore size could compromise both ionic and
osmotic homeostasis, leading to cell necrosis, which may
explain the results obtained in Figure 6. A static pore sizewas
assumed in all calculations to simplify the analysis without
determining the kinetics of the pore, while giving reasonable
estimates of the intracellular concentration. Further experi-
ments examining the effect of intra- and extracellular solute
gradient on pore size and the kinetics of pore formation and
closure is required.
Pore widening has also been observed in electroporation
studies (Kinosita and Tsong, 1977; Tsong, 1991; Weaver,
1993), where membrane potentials exceeding the dielectric
strength of the bilayer resulted in pore expansion. In this
process, the pore expansion was irreversible, since the
resealing time occurred within seconds to minutes (Tsong,
1991) after the pulsewas turned off. This led to compromised
cells, subsequent to the creation of an increased pore size.
Concentration induced stress resulting from the passage of
water through a pore may contribute to decreased cell
survival with increasing extracellular osmolarity. Since the
volume of water inside the cell increases with time, a post-
permeabilized cell could swell to a critical volume, resulting
in cell rupture (Meryman, 1968, 1971). However, the contri-
bution of concentration induced stress at 0.2, 0.3, 0.4, and
0.5 M sucrose is insignificant, as Eroglu et al. reports a pre-
freeze cell survival of 84.1� 3.0% for mammalian cells
porated using a-hemolysin in the presence of 0.4M trehalose
(Eroglu et al., 2000). This is in comparison to a 30� 10%
survival using our permeabilization method, indicating that
an additional competing factor, namely the osmotic rupture
hypothesis (Muldrew and McGann, 1994), is likely respon-
sible for the large deviation in cell survival.
Theoretical Estimates of Intracellular Delivery
Equation (4) was used to estimate the percentage delivery of
intracellular sucrose at equilibrium volume. Figure 7 is a plot
of the solute diffusion profile as a function of distance along
the length of the pore for a cell in 0.2 M sucrose suspension
where tequil¼ 0.2 s. For a cell membrane thickness of L¼10 nm, the accumulation of sucrose was estimated to be
0.199 M. The concentration of 0.199 M is the osmolarity at
the inner surface of the plasma membrane, and does not
represent the final equilibrium concentration at large diffus-
ion lengthswithin the cell. The accumulation of sucrose at the
inner surface of the membrane would diffuse inside the cell,
reducing the overall cytoplasmic sugar concentration. The
inset in Figure 7 is a plot of the sucrose concentration at large
distances within the cell. At x¼ 10 mm, a concentration of
0.145Mwas estimated for cells in 0.2M sucrose suspension,
yielding a loading efficiency of 72.3%. Similar diffusion
plots for cells in 0.3 and 0.5 M sucrose were obtained, with
intracellular sucrose concentrations of 0.198 (0.3 M; 66.0%
loading) and 0.330 M (0.5M; 66% loading). A length of
10 mm was chosen based on the average radius of an MDCK
cell at isotonic volume (presuming a spherical shaped cell).
The amount of intracellular sugar can be controlled based
on the appropriate choice of laser parameters. Using the
modified diffusion equation for a porous membrane, the
solute diffusion constant was assumed to be independent
of the solute concentration. From the continuity equation,
the spatial mass transport rate was converted to a varying
concentration, where Cs (x, t) was solved using initial
conditions (Cs (0, t)¼C0 and Cs (1, t)¼ 0). If we assume
that the diffusion coefficient is not independent of the solute
concentration but linearly proportional to Cs, then D (x,
t)¼DswCs (x, t), where Dsw is the diffusion coefficient of
sucrose inwater,Cs (x, t) is the solute concentration, andD (x,
t) is the modified diffusion constant with linear dependence
on Cs (x, t) (Janavicius and Poskus, 2005). Janavicius and
Poskus (2005) solved the non-linear diffusion equation (for a
non-porous membrane) for a diffusion coefficient directly
proportional to the concentration, and found that the non-
linear equation had a diffusion profile that was smaller in
curvature than the linear diffusion equation. Essentially, the
non-linear equation resembled a linear function, and the
solution to the equation became equal to zero at a certain
distance from the diffusive source (Janavicius and Poskus,
2005). This is in contrast to the linear equation, which
asymptotically approaches zero. Despite these differences,
Janavicius showed that the predicted concentration using the
non-linear equation did not exceed the value predicted by the
linear equation by more than 20% (Janavicius and Poskus,
2005). That is, Cs (x, t) for the non-linear equation was
calculated to be higher than the prediction given by the linear
equation.
A more rigorous definition of Equation (4) would involve
a time component for both the area and length of the pore,
with proper adjustments to the diffusion constant to include
the properties of the cytoplasm. The pore generated by
the focused femtosecond laser pulses is dynamic,with its size
increasing or decreasing with time. This dynamic pore is
different from the static pore created by a-hemolysin and
other bacterial pores (Acker et al., 2003; Eroglu et al., 2000;
Russo et al., 1997). The temporal change in the pore area is
further complicated when described in conjunction with the
osmotic rupture hypothesis, since the area passes through a
maximumand changes in size due to pressure,water flux, and
membrane composition. In our analysis of intracellular
sucrose delivery, we have considered both the area and length
of the pore to be independent of time, without unreasonable
estimates in the percentage delivery (Table I). From Figure 4,
the time taken to reach equilibrium volumewas tequil¼ 0.2 s,
and this led us to conclude that the pore was open for a
duration long enough for the cell to reach this new
KOHLI ET AL.: REVERSIBLE PERMEABILIZATION USING FEMTOSECOND LASERS 897
equilibrium volume. Consequently, the movement of water
was not limited by the time dependence of the pore area and
length. Since the average diameter of a sucrose moleculewas
calculated to be 1.6 nm, with an initial pore diameter of 1 mm,
this alsomeant that the solute fluxwas not limited by the pore
dynamics. On average, based on the ratio of the diameter of
the pore to that of the sucrose molecule, approximately 625
sucrose molecules were calculated to fit across the diameter
of the pore. In relation to Equation (4), Table I, and Figure 7, it
is not surprising to seewhy>98%of the cryoprotectant sugar
diffuses into the cell within less than 270 ms for a distance of
x¼ 10 nm and >70% to a distance of x¼ 10 mm. To further
refine this result, Einstein’s equation for the square of the
average motion of a diffusing particle can be used to estimate
the time required for a single sucrose molecule to diffuse a
predetermined distance x. Choosing the distance to be 10 nm
with Dsw equal to the value given in Table I, t¼ 0.07 ms. So,on average, a single sucrose molecule diffuses to a length of
10 nm in 0.07 ms. If the kinetics of the porewere quicker thanthe mass transport of water, then the calculated value for Cs
(x, t) at the inner surface of the membrane would provide
a concentration value much less than the extracellular
osmolarity. With the average transit time of a sucrose
molecule across the cell membrane being 0.07 ms, the rapidaccumulation of sucrose (>98% for x¼ 10 nm) within
270 ms is expected. Since the intracellular accumulation of
sugar is followed by the movement of water, it is safe to
conclude that both the flux of water and solutes towards
equilibrium volumemust have occurred before the closure of
the pore.
The unique feature of using femtosecond laser pulses
for permeabilizing cells is that the permeation rate for
cytoplasmic uptake of cryoprotectant sugar occurs at a faster
rate than that achieved by other reversible permeabilization
techniques. From Table I, we notice that for each extra-
cellular osmolarity>98% (x¼ 10 nm;>60% for x¼ 10 mm)
sucrose is delivered into the cell within milliseconds. This is
in contrast to 10–15 min required using the a-hemolysin
method (Eroglu et al., 2000), increasing the cell’s exposure
time to the permeabilizing agent.
Maximized Survival Using 0.2 M SucroseResulting From Reversible Optical Pores
Clearly, permeabilization by femtosecond laser pulses has
important consequences for biopreservation applications.
In this study, we have shown that for cryopreservation an
extracellular sucrose concentration of 0.2 M yields the
highest post-permeabilization survival rate. This is not
surprising, as other studies have reported the highest cell
survival using 0.2 M trehalose (Buchanan et al., 2004; Chen
et al., 2001; Eroglu et al., 2000, 2002). The effectiveness of
trehalose and sucrose as cryoprotectants are equal under ideal
conditions (Crowe et al., 2001), and the correlation between
sucrose concentration and cell survival is similar to that
found when using trehalose. Therefore, the choice of using
sucrose or trehalose is completely arbitrary, as both have
been shown to produce similar survival rates (Crowe et al.,
2001).
The Advantages of Femtosecond Lasers
Another benefit of femtosecond laser pulses is that they can
be adapted for precise sub-micron optical perforations
without inducing thermal pressure or shock to the biological
sample. Absorption of high intensity ultrafast laser pulses by
non-linear multiphoton absorption and ionization leads to
multiphoton electronic excitation (Noack and Vogel, 1999),
whereby energy is transported to the liberated electrons
without thermal diffusion to adjacent cellular material
(Chichkov et al., 1996; Loesel et al., 1998; Niemz, 2002).
Since femtosecond pulses are shorter than the thermal
diffusion time (picoseconds to nanoseconds), heat transport
is minimized, and the biological sample remains unaffected
by heat shock and subsequent damage (Loesel et al., 1998;
Niemz, 2002). This effectively renders the reversible perme-
abilization process non-thermal. Therefore, cell damage due
to thermal heating is inconsequential, demonstrating the
advantage of using ultrafast (femtosecond) laser pulses for
reversible permeabilization.
Future Prospects
The application of femtosecond lasers for non-invasive
reversible permeabilization of living cells provides an alter-
native method for achieving the biopreservation of engi-
neered and native cells and tissues. Since post-preservation
survival rates depend on the non-invasive nature of the
permeabilization tool, decreasing the degree of cellular
damage inflicted will inherently increase the preservation
efficiency rate. With the most widely used permeabilization
tools, like electroporation, transient pores irreversibly de-
nature and modify the functional groups of proteins (Tsong,
1991) and compromise cellular function. Therefore, femto-
second lasers provide a significant advancement over current
permeabilizaton techniques.
Furtherwork is being conducted on the post-cryopreserved
survival rate of mammalian cells permeabilized by ultrafast
laser pulses. We anticipate that our study will have important
applications in biopreservation, and expect that this new tool
will impact the preservation of more complicated biological
systems.
The authors would like to thank L.E. McGann and H.Y. Elmoazzen for
their technical expertise in transport equations and cell kinetics, and
H.Y. Elmoazzen, J. Lecak, K.L. Scott, and J.L. Anderson for their
review of this manuscript.
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