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Cite this: Analyst, 2011, 136, 1620
www.rsc.org/analyst PAPER
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Detection of acute brain injury by Raman spectral signature
Li-Lin Tay,*a Roger G. Tremblay,b John Hulse,a Bogdan Zurakowski,b Michael Thompsond andMahmud Bani-Yaghoub*bc
Received 11th November 2010, Accepted 8th February 2011
DOI: 10.1039/c0an00897d
Brain injury can lead to irreversible tissue loss and functional deficit along with significant health care
costs. Raman spectroscopy can be used as a non-invasive technique to provide detailed information on
the molecular composition of diseased and damaged tissues. This technique was used to examine acute
mouse brain injury, focusing on the motor cortex, a region directly involved in controlling execution of
movement. The spectral profile obtained from the injured brain tissue revealed a markedly different
signature, particularly in the amide I and amide III vibrational region when compared to that of healthy
brain tissue. Most noticeably, there was a significant reduction of the amide I vibration at the acute
injury site and the appearance of two distinct features at 1586 and 1618 cm�1. Complementary
immunohistochemical analysis of the injured brain tissue showed an abundant expression of Caspase 3
(a cysteine protease marker used for apoptosis), suggesting that the injury-induced specific Raman
shifts may be correlated with cell death. Taken together, this study demonstrates that Raman
spectroscopy can play an important role in detecting the changes that occur in the injured brain and
provide a possible technology for monitoring the recovery process.
Introduction
Recent years have seen significant advances in chemical detection
science, especially in medicine and the field of clinical diagnos-
tics.1 Techniques involved range from methods for the early
detection of disease to devices designed for point of care, rapid
analyses of biomarkers. A particularly important challenge is
posed by the assessment of brain damage. Injury to this organ is
among the primary causes of death and disability, and is a direct
consequence of irreversible neuronal loss, functional impairment
and limited repair.2,3 The management of brain injury requires
a comprehensive approach in which efficient diagnosis in
combination with an appropriate care and rehabilitation
program may lead to improved recovery. Currently, diagnosis
relies on various imaging techniques in order to complement the
clinical and physiological information acquired at the bedside.
Magnetic resonance imaging (MRI), computerized axial
tomography (CAT) and scanning by positron emission tomog-
raphy (PET) provide significant information concerning changes
aInstitute for Microstructural Sciences, National Research CouncilCanada, Ottawa, Ontario, Canada K1A 0R6. E-mail: [email protected] and Brain Repair, Neurobiology Program, Institute forBiological Sciences, National Research Council Canada, 1200 MontrealRd., Bldg. M-54, Ottawa, Ontario, Canada K1A 0R6. E-mail: [email protected] of Cellular and Molecular Medicine, Faculty of Medicine,University of Ottawa, Ottawa, Ontario, Canada K1H 8M5dDepartment of Chemistry, University of Toronto, 80 St. George Street,Toronto, Ontario, Canada M5S 3H6
1620 | Analyst, 2011, 136, 1620–1626
in brain structure, physiology and metabolic activity caused by
brain damage.4,5 However, the high cost and strict regulation
associated with these systems result in the fact that most hospi-
tals and clinics around the world do not have access to these
technologies. Accordingly, the design and implementation of
a rapid, sensitive, non-invasive and less expensive technique
represent an attractive alternative for diagnostic application.
Moreover, such an advance, even in modern facilities, could lead
to reduced waiting periods and enhancement of the ability of the
physician to reach an early and accurate diagnosis.
To complement the clinically established imaging systems
mentioned above, recent technological advances in optical
techniques provide a promising strategy to obtain valuable
information concerning the brain structure and composition. In
particular, vibrational spectroscopic techniques, such as Fourier
transform infrared absorption spectroscopy (FTIR) and Raman
spectroscopy, are well established methods capable of probing
the distribution and location of biomolecules (proteins, lipids,
nucleic acids) present in the brain and other tissues.6–8 These
techniques provide researchers with a means to study differences
in structure, morphology and chemical composition in tissues
and cells without the need of labels at a sub-cellular spatial
resolution, while being minimally invasive to the cells and tissues
probed. It has been shown that both methods are capable of
discerning healthy from diseased tissues based on biochemical
differences and have been applied to tissue samples from breast,
colon, cervix, skin, liver, lung, brain and from bodily fluids.9–17 In
addition, Raman spectroscopy and FTIR have made contribu-
tions to the field of stem cells by providing a non-invasive
This journal is ª The Royal Society of Chemistry 2011
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approach that complements the label-based histological methods
to determine different cell types.18–21 This is not surprising, since
most samples with displaying disease show fundamental changes
in the biochemistry of the tissue. With respect to the two vibra-
tional techniques, Raman spectroscopy has the added advantage
of higher spatial resolution and insensitivity towards water or
biological buffers making it a particularly suitable method
for probing biological tissues. Raman spectroscopy using mini-
aturized fiber-optic probes could provide clinicians with a
non-invasive means to locate or screen for diseased tissue during
surgical procedures and to monitor post-treatment recovery.
Several reports have been published on the use of the technique
in the study of healthy brain tissues, Alzheimer’s diseased tissue,
and brain tumors.7,17,18,22–29 However, there have been no reports
of the analysis of brain injury by vibrational spectroscopy. In this
paper we present the first Raman spectroscopic analysis of the
brain, using mouse motor cortex injury as a model system. The
spectral fingerprint obtained from injured regions of the brain
has been further complemented by neurobiological measure-
ments in an attempt to provide a correlation between Raman
spectral data and changes in cellular apoptosis observed after
injury.
Experimental procedures
Materials and methods
Tissue preparation. Animal studies were approved by the
Animal Care Committee at the National Research Council
Canada-Institute for Biological Sciences (accredited by the
Canadian Council on Animal Care). Briefly, a total of 16 three-
month-old CD1 mice (Charles River Labs, St Constant, QC)
were anesthetized, using isoflurane (Aerrane, Baxter, Montreal,
QC). The animals were placed into equal ‘‘control’’ (un-injured)
and ‘‘injured’’ groups. To perform an injury, animals were placed
in a stereotaxic frame and the skull was exposed. The injury site
was marked on the bone, using specific coordinates (from ‘‘AP
�0.25 mm to�1.0 mm, Lat +0.7 mm’’, to ‘‘AP +1.25 mm to +3.0
mm, Lat +2.4 mm’’) with respect to Bregma. The bone was
removed with a dental drill, and the motor cortex was injured by
using a sterile needle to remove the neural tissue at a depth of 1
mm. Animals were sacrificed right after injury (along with their
control counterparts), and the whole brain was removed, washed
and maintained in Hank’s Balanced Salt Solution (HBSS, Invi-
trogen, Mississauga, ON), and immediately examined by Raman
spectroscopy. In parallel experiments, horizontal sections were
prepared and deposited on a microscope slide (8 mm thick
sections for immunohistochemistry) according to previously
established procedure.30
Immunohistochemistry. Mouse brains were fixed with 10%
formalin for 16 hours, processed (Thermo Shandon, Citadel
1000, Pacific Southwest Lab Equipment Inc., Vista, CA, USA)
and paraffin-embedded (Thermo Shandon Histocentre 2, Pacific
Southwest Lab Equipment Inc.). Each brain sample was
sectioned into 8 mm slices (Leica RM2165 Microtome, Ger-
many), after which the sections were de-waxed with xylene (5
minutes in each of the three sequential baths), hydrated in
ethanol (100%, 90%, 70%, and 50% for 5 minutes each), and
This journal is ª The Royal Society of Chemistry 2011
washed with phosphate buffered saline (PBS, three times for 5
minutes).30 Sections were incubated with polyclonal Caspase 3
antibody (Santa Cruz, CA, USA, diluted 1 : 50 in 1% BSA) and
monoclonal microtubule associate protein 2a + 2b (MAP2, clone
AP-20, 1 : 200, Sigma, Toronto, ON, Canada) or glial fibrillary
acidic protein (GFAP, clone GA-5, 1:100, Neomarkers, Fre-
mont, CA, USA) for 1 hour at room temperature, washed with
PBS (three times, 10 minutes each) and labeled with Alexa-
conjugated anti-rabbit IgG (Invitrogen, Mississauga, ON, Can-
ada, diluted 1 : 600 in 1% BSA) and rhodamine-conjugated anti-
mouse IgG (1 : 600; Jackson Immunoresearch Laboratories) for
1 hour. Sections were washed again with PBS (three times, 10
minutes each), stained with Hoechst (Invitrogen, Eugene, Ore-
gon, USA, 1 mg ml�1) for 10 minutes, rinsed with water and
covered with Vectashield mounting medium (Vector Laborato-
ries, Burlingame, CA). The immunoreactivity was examined with
an Axiovert 200M fluorescence microscope, AxioCam and Axi-
ovision 4.7.2 (Zeiss, Germany). The images were processed with
Adobe PhotoShop (Adobe Systems Incorporated, Mountain
View, CA) and CorelDraw (Corel Corporation, Ottawa, ON).
Raman spectroscopy. Raman spectroscopy was performed
with a commercial microRaman system (LabRAM HR, Horiba
Jobin Yvon, Edison, NJ) equipped with a software controlled
XY stage and a thermal-electric cooled CCD detector. Samples
(whole mouse brain) were excited with 785 nm single mode diode
laser (XTRA, Toptica Photonics Inc., Victor, NY) at a power
density of �104 W cm�2 without having problems such as auto-
fluoresence.29 Incident radiation was coupled into an Olympus
BX51 optical microscope and focused to �4 mm diameter spot
through a Leica 50� long working distance objective. Whole
brain samples were placed on a microscope slide and irradiated
through the microscope objective (NA: 0.55). Backscattered
Raman emission was collected by the same objective with an
8 second integration time and dispersed with a 300 groove per
mm grating. Rayleigh rejection was achieved with a notch filter.
For the un-fixed tissue samples, all Raman measurements were
started immediately following the removal of the brains from the
skull and completed within one hour of the surgery.
Results and discussions
Although Raman spectroscopy is a particularly well-established
technique, it is an emerging diagnostic tool when it comes to the
early detection of chemistry associated with diseased tissues. The
method displays considerable potential due to its sensitivity to
molecular composition, and to structural conformational
changes associated with pathological features that cannot be
detected easily by conventional morphological methods. Most
previous Raman studies of brain tissue have been performed
either on frozen or fixed tissue cross-sections. While frozen
tissues are commonly employed in vibrational studies, the
complicated handling process can significantly reduce the
experimental flexibility. On the other hand, the fixation process
needs to be carefully performed to facilitate the proper
interpretation of experimental results.31 Real-time chemical
information can be obtained from living cells by performing
in situ monitoring of samples.20,29 In the latter report, bleeding
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artifacts were avoided partially by injecting cancer cells through
the carotid artery to form tumors in the mouse brain.
In our study the injury was mechanically introduced to the
motor cortex through a cranial window (and meninges),
a phenomenon observed in the patients with brain injury caused
by motor vehicle accidents, penetration of foreign bodies into the
neural tissue or tumor excision during surgical procedures.32 We
performed Raman spectroscopy on the healthy and injured
motor cortices immediately after the whole brain was removed
from the skull. Additionally, parallel immunohistology experi-
ments were also done on the fixed brain samples to enable critical
comparison with the Raman spectral features introduced by
injury. With prior expertise established in neuroregeneration,32
we have used a focal brain injury mouse model system that
Fig. 1 The images of control and injured adult mouse brains. The high
resolution digital photographs (A and D) and optical images (B and E)
show significant differences between the healthy (A–C) and injured (D–F)
brains. The injury was mechanically introduced to the left motor cortex
(D, circled). Corresponding immunohistochemical images reveal intact
neurons (arrowheads) in the healthy motor cortex (C). In contrast,
neurons are significantly affected by injury, as evidenced by morpho-
logical features and MAP2 immunoreactivity (F). Cb: cerebellum, Ncx:
neocortex, and OB: olfactory bulb. Scale bar: A and D (1.6 mm), B and
E (400 mm), C and F (70 mm).
1622 | Analyst, 2011, 136, 1620–1626
mimics human conditions33 and allows controlling the injury size
in a reproducible and quantifiable manner (Fig. 1). The injury
was introduced to the left motor cortex (Fig. 1D) and compared
to its counterpart in the right hemisphere (as internal control in
the same mouse) and the left motor cortex in the control mice
(Fig. 1A). Optical images of the healthy (Fig. 1B) and injured
(Fig. 1E) motor cortices as seen under the optical microscope
showed significant discolouration in the injured sites (Fig. 1E) as
a result of mechanical damage to the tissue. The regions exam-
ined spectroscopically were further evaluated by fluorescence
microscopy (Fig. 1C and F) to correlate the changes in the
injured area at the cellular level. Fig. 1C shows well-organized
MAP2 positive neuronal cell bodies and dendrites in the healthy
motor cortex, whereas, the injured motor cortex (Fig. 1F)
exhibited significant tissue loss as well as damage to the cell
bodies and neurite extensions in the vicinity of the injury core.
Raman spectroscopy of fresh and fixed brain samples
Fig. 2 presents a series of typical Raman spectra from eight intact
motor cortices. Spectra 1–4 were obtained from fixed tissue
samples, whereas, spectra 5–8 were acquired from fresh tissues.
All freshly prepared (un-fixed) samples were maintained in the
physiological buffer (HBSS) and applied to spectroscopic studies
immediately after the surgical procedure.
Both fresh and fixed samples exhibit a strong band at 1660
cm�1, that is attributed to the amide I vibration of the protein and
C]C stretching of lipids. Three broad features at 1274, 1301 and
1346 cm�1 are also obvious in both sets and are attributed to the
amide III vibration of protein and CH deformation of protein
Fig. 2 Raman spectroscopy of fresh and fixed healthy adult mouse
brains. Consistent peaks (1002, 1274, 1450 and 1660 cm�1) are present in
the spectra obtained from both fixed (1–4) and fresh (5–8) brain samples.
All spectra were obtained with 785 nm excitation radiation.
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and lipid components in the probed tissue. The sharp and narrow
feature at 1002 cm�1 is associated with the ring breathing mode of
phenylalanine in the protein. The series of bands at 1033, 1090
and 1130 cm�1 are attributed to the C–N stretch of phenylala-
nine, the PO2� stretch of phospholipids and nucleic acid, and the
C–C stretch, respectively. The sharp and strong band centered at
1450 cm�1 is assigned to the CH2 deformation mode from both
lipids and proteins. In addition, in the un-fixed samples (spectra
5–8, Fig. 2), a small band at 1740 cm�1 due to the carbonyl
stretch of the ester group of the lipids is also observed. These
observations are in agreement with the earlier studies of mouse,
rat and human brains.22,23,26,27,29 A comparative analysis shows
several common spectral signatures (such as 1002, 1090, 1130,
1274, 1450 and 1660 cm�1) in the fresh and fixed tissues.
However, there are intriguing differences between the two sets of
data, likely due to fixation and its consequent delipidation.
Specifically, the C–N stretch of phenylalanine (1033 cm�1) and
the lipid carbonyl stretch at 1740 cm�1 are consistently different
between the fresh and fixed samples. Spectra obtained from the
fresh tissues generally show a 1033 cm�1 band, but upon fixation,
this band weakened. The fixed samples also consistently show
a decrease or disappearance of the 1740 cm�1 band compared to
the fresh tissues possibly due to delipidation during the fixation
process.24 Since the brain tissue, in particular white matter,
contains high (5–15%) lipid content2 and various structural
proteins, the adjunct Raman spectroscopy of fresh and fixed
samples provided an appreciation of the differences between the
two methods used to prepare brain samples. Such comparison is
essential with respect to an accurate discernment of the spectral
fingerprint of brain injury from changes caused by sample
preparation.
Spectral signatures of healthy and injured brain tissues
Through the comparative studies of fresh and fixed brain
samples, we were able to establish that the fixation process did
not impact the major vibrational signatures. Therefore, we used
both fresh and fixed brain tissues to examine the effect(s) of
Fig. 3 Comparative Raman spectroscopy of healthy and injured adult mo
cortices demonstrate consistent Raman shifts following injury.
This journal is ª The Royal Society of Chemistry 2011
injury by Raman spectroscopy. Two sets of control brain
samples were used to compare with the injured region: the
healthy brains obtained from the uninjured mice and the
contralateral (opposite) motor cortex from the injured mice.
The latter serves as the most appropriate control for organs such
as the brain, which contain two structurally symmetric hemi-
spheres. Fig. 3 shows marked differences in the Raman spectra
obtained from the control (Fig. 3A) and injured (Fig. 3B)
hemisphere of six independent mice. Most notably, the charac-
teristic amide I vibration at 1660 cm�1, one of the most prom-
inent features observed from all control brain samples, was much
weaker in the spectra obtained from the injured brain samples.
Instead, two sharp bands located at 1586 and 1618 cm�1 appear.
The observed differences appear to be weakly correlated with the
sharp phenylalanine modes at 1002 cm�1. In the spectra taken
from the injured site (Fig. 3B), the band at 1002 cm�1 was either
weak or absent, as compared to the strong feature observed in
the undamaged hemisphere (Fig. 3A). Furthermore, the peak
structure in the region of the amide III vibration changes
significantly and two additional bands at 1175 and 1227 cm�1 are
observed in spectra obtained from the injured site. These features
resemble the vibrational features that are characteristic of
cholesterol and phospholipids.34 There is evidence that addi-
tional bands (such as minor Raman bands at 750, 1002, 1212,
1546, 1605 and 1619 cm�1) can be produced due to the resonance
excitation of the haemoglobin, resulting in increased Raman
cross-sections of heme-associated vibrations.29 In our study, we
have taken extra care to ensure that robust and reproducible data
are obtained from multiple brain samples. A similar ex vivo
approach has been taken by others to establish Raman maps of
brain specimen. In particular, many of the spectral features
obtained from the brain in our study are similar to those
previously reported,7 further validating the use of ex vivo brain
samples for Raman spectroscopy. In addition, Raman spec-
troscopy of ex vivo brain samples has been sufficient to demon-
strate that human intracranial tumours such as gliomas have
more haemoglobin and lower lipid to protein rations, and
meningeomas contain more collagen than normal brain tissue.7
use brains. Raman spectra from the control (A) and injured (B) motor
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One of the techniques that can play a major role in the
improvement of detection sensitivity is surface-enhanced Raman
scattering (SERS).35–37 It is well-known that living cells can
uptake and transport nanoparticles through an endosomal
pathway through which nanoparticle aggregates can produce
large spectroscopic enhancements used for analysis by SERS.38
In fact, multi-color SERS nanotags have been used to detect
tumour cells expressing epidermal growth factor receptor
(EGFR) or other cell surface receptors as well as identification of
pathogenic microorganisms.36,39–44 The SERS nanotags are
typically made of Raman reporter molecules, with gold nano-
particles encapsulated in a protective SiO2 or polymer shell,
functionalized with antibodies of interest for targeted molecular
imaging. In addition, others have used SERS to distinguish the
spectra between healthy and tumour samples,45 by sudden
freezing of tissue in liquid nitrogen followed by crashing and
mixing the sample with a concentrated silver colloidal suspen-
sion. More recently, SERS has been used to monitor the chemical
changes that occur during differentiation of human adipose
derived adult stem cells.20 However, despite its above-mentioned
applications, the delivery of SERS active nanostructures into the
injury site (without altering the local biochemistry) remains
a great challenge.46–48 SERS holds amazing promises to all forms
of Raman spectroscopy and it can certainly be integrated in this
study, if the presence of metallic nanostructures does not pose
changes such as photothermal reactions to the injury state of the
tissue.
Since the motor cortex is composed of six distinctive layers
(layers I to VI), it is possible that removal of the outermost
portion of the cortex (layers I and II) allows the detection of
molecular signature of lower layers (layers III and IV) by Raman
spectroscopy. However, if this is the case, cross-sectional studies
of brain tissues should reveal such differences. The second
possible explanation for the observed spectral difference in our
study is the change in biochemical composition of the probed site
induced by the injury itself. To evaluate such a possibility, we
carried out immunohistology in the tissue sections in order to
understand the observed spectral differences.
Fig. 4 Caspase 3 activity in the control and injured adult mouse brains.
(A) Histological analysis of healthy brains shows almost no Caspase
3 immunoreactivity in the control motor cortex. (B) A corresponding
phase contrast image confirms a normal cortical structure. (C) The
injured motor cortex reveals an abundant level of Caspase 3 protein
within the cell bodies. (D) The abnormal cell bodies (arrowheads) can be
also detected in the corresponding phase contrast image. (E) MAP2
immunostaining shows that most Caspase 3 positive cells (C) are neurons.
(F) Bar graph depicts the percentage of Caspase 3 positive cells in
neurons and astrocytes in comparison to the control samples. Scale
bar: 15 mm; p < 0.001, one-way ANOVA.
Immunohistology of the injured brain
Raman microspectroscopic mapping of apoptotic cells such as
lung fibroblasts and lung carcinoma epithelial cells has demon-
strated fragmentation of the nucleus, degradation of proteins,
disappearance of lipid bodies and reduction in the intensity of
nucleic acid bands.49,50 Furthermore, other reports have shown
that traumatic brain injury and stroke cause cell death in the
damaged tissue,51 however, the observed injury-induced Raman
spectral features (1586 and 1618 cm�1) have neither been repor-
ted nor assigned. Therefore, it is unclear what biomolecular
activities in the injured region would be responsible for this
observation. One possible hint was provided by the recent
Raman studies from sub-cellular components and other
immortal cell lines, suggesting that the new Raman bands
observed in these cases (1560 to 1640 cm�1) are closely associated
with the mitochondrial activity of cells.52–54 Interestingly, mito-
chondria generate most of the energy of the cell in the form of
adenosine triphosphate (ATP) and are involved in several
processes, such as signaling and cell death. Therefore, it is
1624 | Analyst, 2011, 136, 1620–1626
possible that the new Raman bands observed in this study may
be linked to mitochondrial activity and ultimately to cell death. It
is known that as a natural response to injury, glial cells occupy
the damaged region (gliosis) and form the glial scar. However,
since the formation of glial scars take at least several days, this
process is unlikely to be associated with the observed spectral
difference obtained immediately following the injury. It is well
known that cerebral ischemia triggers two general pathways of
apoptosis: the intrinsic pathway, originating from mitochondrial
release of cytochrome C, which is associated with stimulation of
Caspase 3; and the extrinsic pathway, originating from the
activation of cell surface death receptors, resulting in the stim-
ulation of Caspase 8.55 In particular, Caspase 3 has been shown
to be activated by mitochondria upon cellular apoptosis in the
brain and other tissues.56 Thus, a comprehensive immunohisto-
chemistry analysis was performed to determine the percentage of
Caspase 3 positive cells in the normal and injured tissues. The
Caspase 3 immunofluorescence image of the normal tissue shows
a low level of Caspase 3 protein (Fig. 4A), while the image
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obtained from injured tissue reveals a significant number of cells
with high Caspase 3 levels (Fig. 4C). Furthermore, Caspase 3 was
used in combination with either a neuronal (MAP2) or astrocytic
(GFAP) marker to determine the identity of Caspase 3 positive
cells. Fig. 4E shows the corresponding MAP2 immunofluores-
cence image of the same injured region also stained with Caspase
3 (Fig. 4C). In addition, phase contrast optical images of the
injured tissue revealed abnormal cell bodies (Fig. 4D, arrow-
heads), which are absent in the normal tissue (Fig. 4B). Using
double staining with either Caspase 3 and MAP2 or Caspase 3
and GFAP, we were able to determine the percentage of the
neurons and astrocytes that were positive for Caspase 3 in
normal and injured tissues and summarize the percentage of
Caspase 3 positive cells. Fig. 4F shows that there is a negligible
percentage (less than 5%) of Caspase 3 positive neurons in the
normal tissue, whereas the majority (>90%) of neurons in the
damaged tissue express Caspase 3. The Caspase 3 expression
levels from the injured tissues suggest that the early apoptotic
events occur mainly in neurons, as most astrocytes in both
normal and damaged tissues are Caspase 3 negative (Fig. 4F).
Thus, neurons appear to be, at least initially, more susceptible to
injury-induced cell death than astrocytic glial cells at this stage.
These results are in agreement with an earlier report, which
demonstrated that multiple Caspases are activated after trau-
matic brain injury.51 Since cortical injuries may quickly lead to
alterations in cerebral energy metabolism including reduced
ATP, GTP and nicotinic enzymes,57 the Raman shifts observed
in this study are thought to correlate to changes in the energy
level following injury associated with the altered mitochondrial
activities in the localized tissues. While an upregulation of
cytochrome C and Caspase 3 may account for some of the
changes observed in the spectra observed after injury, it remains
to be elucidated whether mitochondria are the first target in this
phenomenon or whether they are only affected indirectly. An
alternative approach to resolve this issue would be to examine
other cellular organelles along with mitochondria by electron
microscopy.
Conclusions
In this study, distinct reproducible features observed in the
acquired Raman spectra were compared between control and
injured brains. The Raman spectroscopic signature obtained
from the injured brain consistently reveals significant spectral
differences in the amide I vibrational region with a reduction of
the intensity of amide I band concomitant with the appearance
of additional features at 1587 and 1618 cm�1. The observed
differences show correlations with the sharp phenylalanine
modes at 1002 cm�1, which was either weak or absent from the
spectra obtained from the injury site. We employed Caspase
3 immunohistochemistry to establish a possible link between the
observed Raman signatures from the acute injury tissues and
apoptosis. This study provides the first observation of such
significant difference in the spectroscopic signature from the
acute brain injury and serves as a baseline for future studies on
acute and chronic injuries of the central nervous system. There is
no doubt that our study can further benefit from methods such as
principal component analysis (PCA) and linear discriminant
analysis (LDA) for spectral comparisons.16,18,19,58 Combined
This journal is ª The Royal Society of Chemistry 2011
PCA-LDA has been used by different laboratories to distinguish
cell types such as stem cells, transit amplifying cells and
terminally differentiated cells in the corneal epithelium,18 stem
cell region of human intestinal crypts,19 and distinct zones in
normal and tumour prostate samples.16,58 In our future studies,
we will take advantage of PCA-LDA to further analyze the
biochemical differences associated with injury and to evaluate
the cell types present in the injured region during acute and
chronic phases.
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