Mathematical modeling of thin-layer drying of fermented and non-fermented sugarcane bagasse
Characterization of sugarcane bagasse by autofluorescence microscopy
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Transcript of Characterization of sugarcane bagasse by autofluorescence microscopy
ORIGINAL PAPER
Characterization of sugarcane bagasse by autofluorescencemicroscopy
Tiago A. Chimenez • Marcelo H. Gehlen •
Karen Marabezi • Antonio A. S. Curvelo
Received: 13 March 2013 / Accepted: 27 November 2013
� Springer Science+Business Media Dordrecht 2013
Abstract The spatial distribution of chemical com-
pounds in sugarcane bagasse is an important issue in
its use as a raw material for second generation ethanol
production from cellulose hydrolysis. Lignocellulosic
materials including whole bagasse, fiber, pith, and
respective samples obtained after chemical bleaching
were investigated using confocal fluorescence micros-
copy and spectroscopy with one and two-photon
excitation. Autofluorescence from unbleached sam-
ples revealed that emission from fiber walls containing
the lignin fraction was longitudinally oriented. After
bleaching treatment, the oriented emission was par-
tially disrupted. Autofluorescence from bleached
samples with a residual lignin content of about 1 %
was ascribed to improved dispersion of remaining
fluorophores throughout the samples inducing a con-
comitant reduction of fluorescence self-quenching in
the samples. The combination of autofluorescence
images with spectral emission and lifetime measure-
ments provides a tool for microscopic characterization
of natural bagasse samples. Moreover, the technique
allows monitoring bleaching processes related to
lignin removal.
Keywords Autofluorescence � Fluorescence
microscopy � Sugarcane bagasse � Lignin
Introduction
The global use of ethanol as a biofuel has expanded its
production from different natural resources (Farrell
et al. 2006). Sugarcane is one of the most common
feedstocks used to produce ethanol (Goldemberg
2007). In the production of ethanol from sugarcane
using fermentation, the total sugar represents only
12–17 % of the wet weight of the plant (Wheals et al.
1999). The solid material produced left after sugarcane
processing is called bagasse and it contains cellulose
(34–47 %), polyoses (24–29 %), and lignin
(18–28 %) (Nassar et al. 1996; Aguilar et al. 2002;
Gray 2007).
Bagasse is usually burned in boilers for steam
production and cogeneration of electricity, but it may
also be used for production of cellulosic ethanol
(Emsley 2008). The chemical or biochemical hydro-
lysis of cellulose from bagasse can be improved by
better knowledge of the micromorphology, chemical
composition and interaction of bagasse with different
biomacromolecules (Sant’Anna et al. 2013).
The dispersion of lignin and other related com-
pounds in the cellulose matrix can provide different
T. A. Chimenez � M. H. Gehlen (&) � K. Marabezi �A. A. S. Curvelo
Instituto de Quımica de Sao Carlos, Universidade de Sao
Paulo, Sao Carlos, SP 13560-590, Brazil
e-mail: [email protected]
K. Marabezi � A. A. S. Curvelo
Laboratorio Nacional de Ciencia e Tecnologia do
Bioetanol, CTBE, Campinas, Brazil
123
Cellulose
DOI 10.1007/s10570-013-0135-9
features of the material including its recalcitrance and
the applications of the material. The distribution of
cellulose and lignin in plant tissues has been investi-
gated using different methods (Parameswaran and
Liese 1982; Daniel et al. 1991; Saka and Goring 1988;
Westermark et al. 1988; He and Terashima 1991; Li
et al. 2012).
There are also some specific methods to recognize
compounds within the cell walls of wood, such as
carbohydrate-binding modules (Joseleau et al. 2004),
most of which use molecular probes to stain specific
components (Vazquez-Cooz and Meyer 2002). Light
microscopy using dyes is a useful way to identify and
localize the presence of lignocellulosic compounds in
raw materials, and possesses the advantages of being
non-invasive and non-destructive (Konig 2000; Zhu
et al. 2011). In particular, the dye safranine has been
used to stain lignin in plant tissue and cellulose fibers
(Horobin 2002; Vazquez-Cooz and Meyer 2002; Bond
et al. 2008). Sugarcane bagasse is a complex material in
which different compounds should influence fluores-
cence its properties. Therefore studies using autofluo-
rescence has seldom been explored in conjunction or
with fluorescent dyes in order to get more information
about the system (Bond et al. 2008). On the other hand
authors have employed fluorescence lifetime imaging
microscopy (FLIM) related to lignin autofluorescence
to map its distribution in samples of sugarcane bagasse
and establishing relationship between lifetimes with
bleaching treatments (Coletta et al. 2013).
The autofluorescence of natural cellulose fibers has
been assigned to the presence of lignin fractions and
aromatic compounds, such as lignans, flavonoids and
tannins, found in the plant cell wall (Olmstead and
Gray 1993, 1997; Konya and Scaiano 1994; Albinsson
et al. 1999). Other researchers have ascribed this
fluorescence to the presence of nicotinamide adenine
dinucleotide in reduced form, flavins such as flavin
adenine dinucleotide, flavin mononucleotide and fla-
voproteins (Schwille et al. 1999). Studies of monocot
cells by ultraviolet fluorescence microscopy demon-
strated that the emission from natural phenolic acids in
the cell wall depends on sample pH (Harris and
Hartley 1976, 1980). Overall, several compounds may
be responsible for the autofluorescence of raw cellu-
lose fibers (Castellan et al. 2007).
Light microscopy has enlarged the scope for
investigation of cell walls (Perera et al. 2011; Harter
et al. 2012). In this context, confocal laser scanning
microscopy (CLSM) has allowed autofluorescence
images with resolution down to 400 nm and morpho-
logic features in two and three dimensions to be
obtained.
Studies exploiting the autofluorescence properties
of plant tissue and natural fibers have been performed
using fluorescence intensity imaging (Wuyts et al.
2010; Jaedicke et al. 2011). However, to identify
components using dye labeling or autofluorescence of
cellulosic materials, additional emission parameters
should be measured. Fluorescence intensity images
and local fluorescence decay profiles may be obtained
by multiphoton excitation using short laser pulses
(Cheng et al. 2001). Multiphoton excitation enhances
the depth resolution compared with that of normal
laser excitation (Denk et al. 1990). Such characteriza-
tion may allow sugarcane bagasse to be studied from a
microscopic point of view.
In this contribution, sugarcane bagasse, fiber and
pith are studied by confocal fluorescence microscopy
with one and two-photon excitation. The autofluores-
cence and dye emission from samples containing
added safranine are measured at steady-state and
under time-resolved conditions. Our goal is to evaluate
the efficiency of chemical bleaching to decompose and
remove lignin from natural cellulosic raw materials.
Experimental
Preparation of sugarcane bagasse samples
The bagasse was washed in distilled water to remove
impurities such as soil and dust. The same procedure
was also used to separate fiber and pith fractions by
wet depithing under a jet of water. A sieve system
consisting of 16 and 60 mesh screens was used to
separate the bagasse. Fiber was retained on the 16
mesh screen, while pith was washed through to the 60
mesh one. Extractives were removed by exhaustive
extraction in two sequential steps using cyclohexane/
ethanol (1:1, v/v) and then water.
Oxidative delignification was performed using dry
sample (whole bagasse, fiber or pith, 3 g) that was free
of extractives. The sample was placed in a 250 mL
three-neck round-bottomed flask containing distilled
water (160 mL). Glacial acetic acid (0.6 mL) and
sodium chlorite (1.88 g) were then added to the stirred
suspension. Delignification was performed at
Cellulose
123
70–80 �C and pH 4 for 3 h according to the optimal
parameters of Browning (1967). Further measures of
glacial acetic acid and sodium chlorite were added
every hour.
The standard method (Browning (1967) used to
evaluate total polysaccharides (holocellulose) in bio-
mass was modified to take into account the oxidation
step used to remove the lignin fraction from the natural
samples. The weight loss obtained by oxidation was
compared with the amount of lignin in unbleached
samples determined previously using the Klason
method. Typically, the percent fractions of holocellu-
lose and lignin in the natural samples were: whole
bagasse (79.9 and 20.1 %, respectively); fiber (76.7
and 22.3 %, respectively) and pith (79.2 and 20.8 %,
respectively). The content of polysaccharides obtained
after bleaching corresponds to the total polysaccharide
determined to be in the original samples. The bleach-
ing stage produced samples containing\1 % residual
lignin. The crystallinity of whole bagasse was deter-
mined by X-ray diffraction (XRD) on a Rigaku
UltraX-18HF rotating-anode generator with Cu Karadiation (k = 1.54 A). The experimental setup used
here was described by Driemeier and Calligaris
(2011), Driemeier et al. (2011). The crystallinity of
the bagasse sample was 0.55 g/g. Pulps derived from
bagasse using different pulping procedures are
reported to possess crystallinities of 0.59–0.78 g/g
(Driemeier et al. 2011). This increase in crystallinity is
caused by the removal of lignin enriching the fraction
of cellulose in the samples.
Safranine staining
Whole bagasse and bleached whole bagasse (BWB)
samples (5 g) were stained by immersion in an
aqueous solution of safranine (3 9 10-5 mol/L) for
5 min. Samples were then rinsed three times for
10 min each in warm water at 40 �C.
Scanning electron microscopy (SEM)
Sugarcane bagasse SEM images were obtained using a
microscope (LEO, 440) with an Oxford detector at an
accelerating voltage of 20 kV. The dried samples were
deposited on a carbon tape and covered with a 4 nm
gold layer.
Fluorescence microscopy
Fluorescence images were obtained using a plate
scanning confocal microscope setup. The custom-
made instrument was based on a microscope (Olym-
pus IX71) with a digital piezoelectric controller and
stage (PI, E-710.3CD and P-517.3CD) for nanometric
sample scanning. The excitation source was continu-
ous wave diode lasers (Coherent Cube, 405 nm), with
an operating at a low power producing \1 mW over
the samples. The excitation beam was converted into a
circularly polarized laser beam using zero-order
quarter-wave plates (Del Mar Photonics) and focused
on the sample with an objective (Olympus, UPLFLN
40X). The emission signal was separated from the
laser excitation beam using a dichroic cube (Chroma,
z405lp) and notch filter (Semrock, NF02-405U-25). In
two-photon excitation, an 800-nm mode-locked beam
with pulses of 150 fs from a Ti: sapphire laser (Mira
900) pumped by a coherent laser (Verdi, 5 W) was
used. The laser pulse frequency was reduced to 4 MHz
using a pulse picker (Conoptics). A dichroic cube
(Chroma, E750sp-2p with 700dcspxr) and notch filter
(Semrock, NF01-808U-25) were used in the confocal
line of the microscope in two-photon excitation
experiments. Photons were counted using an ava-
lanche photodiode point detector (Perkin Elmer,
SPCM-AQR-14) aligned with an 80-lm pinhole in
the confocal line. Transistor-transistor logic detector
signals were collected with a counter/timer peripheral
component interconnect card (NI 6601) and trans-
ferred to a personal computer for 2D plotting using a
scanning control program written in C#. Fluorescence
decays were measured by a single-photon timing
technique using a counting board (Becker and Hickl
140) with start laser pulses triggered by a photodiode
(PicoQuant TDA 200). Decays were analyzed by
multiexponential fitting without deconvolution using
the FAST software (Edinburgh Instruments).
Samples measured by fluorescence microscopy
were added to ethanol and briefly subjected to low
power ultrasound to disperse particles. Dry bagasse
samples were supported in a glass-bottomed Petri dish
(35 9 10 mm, 1.5, Ted Pella). Samples showed a
wide range in length (100–600 lm) and width
(20–100 lm). Fluorescence images covering a square
region of 60 9 60 lm with a pixel size of 200 nm
were recorded using false-color mapping, reaching the
best contrast enhancement according to the difference
Cellulose
123
in intensity of the fluorescence signal. Hereafter, the
position of a given emission spot was recovered for
spectral emission decay measurements. Only spots
with almost constant and high photon emission rate
indicating low or negligible damage caused by
photobleaching were further analyzed. Emission spec-
tra were obtained using a spectrometer (Maya 2000
Pro, Ocean Optics) coupled with a fiber to the
binocular side port of the Olympus IX71 microscope.
A long pass filter (Thorlabs, cut-off wavelength of
450 nm) was used to avoid the excitation light. The
emission spectrum of microcrystalline cellulose (Avi-
cel� PH-101, Sigma-Aldrich) was also measured for
comparison with those obtained for sugarcane
bagasse.
Results and discussion
SEM analysis of sugarcane bagasse samples (whole
bagasse, fiber and pith), and the corresponding
bleached samples (BWB, bleached fiber (BF) and
bleached pith (BP)) was used to determine the effect of
chemical bleaching. These regions were analyzed
because they present unique characteristics with
respect to their recalcitrance and morphology. Integral
bagasse consists of fiber and pith. The fiber surface is
formed by parallel stripes and has a high rate length/
diameter. In contrast, pith has a fragile and fragmented
structure correspondent to parenchyma cells designed
to store sucrose. These features are very important to
carry out hydrolysis and bleaching processes. In Fig. 1
SEM compares micrographs of unbleached and
bleached samples. Unbleached samples (Fig. 1a, b,
c) present a rigid and compact morphology. After
chemical bleaching, fiber and pith exhibited a more
disorganized morphology. The roughness increased in
the surfaces and some microsized splinters were
observed (Fig. 1d, e, f). Therefore, after bleaching,
samples showed most exposed structure, which allows
more accessibility hydrolysis reaction of lignocellu-
losic biomass (Novaes et al. 2012).
Fig. 1 SEM images of bagasse samples: a whole bagasse, b fiber, c pith, d BWB, e BF and f BP. Microsized splinters are indicated by
arrows in samples after bleaching process
Cellulose
123
Autofluorescence images of treated and untreated
sugarcane bagasse samples were performed to study of
morphological microenvironment in cellulose matrix
and to evaluate distribution of lignin fraction before
and after bleaching process.
Confocal fluorescence images of whole bagasse,
pith and fiber sample, and the corresponding bleached
samples BWB, BF and BP obtained by single-photon
excitation at 405 nm, are compared in Fig. 2. The
material absorbs light in a wide spectral range, from
the near ultraviolet to the visible, due to their
complexity and microenvironmental diversity. How-
ever, the samples showed higher emission intensity
when excited at 405 nm region. All samples exhibit
quite strong autofluorescence without fine structure. In
other words it is not possible shows the individual dots
that form the structure. Therefore, well oriented
straight row tracks structures formed by the longitu-
dinal organization of fibers do not appear in any region
observed in both natural and bleached samples.
Autofluorescence arises from compounds dispersed
in the walls of the plant cells (Harter et al. 2012),
mostly from the lignin fraction. Features related to
structure and thickness affect resolution and contrast
of fluorescence images. In addition, the excitation
light at UV–Vis region cause scattering in the samples,
and conventional confocal microscopy study of plant
tissues may be limited by the opacity of the medium.
(Cheng et al. 2000a; Benediktyova and Nedbal 2009).
This problem can be overcome by using two-photon
microscopy, because scattering and absorption are
substantially reduced in the near-infrared range com-
pared with in the visible (Denk et al. 1990; Cheng et al.
1998).
Images of sugarcane cellulose materials measured
by two-photon microscopy are illustrated in Fig. 3.
The images show greater structural detail compared
with images obtained using conventional confocal
microscopy. In addition, images generated from two-
photon excitation contained some microstructure
information and more detailed fluorescence mapping
than single-photon excitation images. Two-photon
Fig. 2 Fluorescence microscope images of a whole bagasse, b fiber, c pith, d BWB, e BF and f BP. Samples were excited at 405 nm.
Scale bar 10 lm. The lateral color scale bars are related to the fluorescence intensity
Cellulose
123
Fig. 3 Fluorescence intensity image and decay traces of
indicated emission spots obtained by two-photon excitation at
800 nm of a whole bagasse, b fiber, c pith, and corresponding
bleached samples, d BWB, e BF and f BP. Scale bar 10 lm.
Decay fitting parameters are given in Table 1. The lateral color
scale bars are related to the fluorescence intensity. Oriented
fluorescence tracks are indicated by arrows in a whole bagasse,
b fiber
Cellulose
123
microscopy can give supplementary characterization
of lignocellulosic materials (Cheng et al. 2000a, b),
because transitions between states of the same parity
are forbidden for one-photon excitation, but they are
allowed for the two-photon excitation (Callis 1993).
The fluorescence images in Fig. 3 show sequences
of small fluorescence spots that form well oriented
straight row tracks, which are related to lignin fraction,
especially from unbleached whole bagasse and fiber
samples. The average distance between two oriented
fluorescence tracks is about 12 lm, which is compa-
rable with the distance between cell walls determined
by SEM (see Fig. 1b). Fluorescence spots in pith
samples show a decrease in intensity and disordered
structure, it does not generate straight tracks format.
In contrast to untreated samples, images of
bleached samples do not contain emission tracks;
instead, some blurry emission spots are evident. This
result is consistent with disorder increasing in the
samples after chemical bleaching because of disper-
sion of crystalline cellulose domains.
Scanning the z position of the focal plane using two-
photon fluorescence microscopy allowed us to visu-
alize the architecture, fibril patterns, and other details
of the microstructure of cellulosic materials displaying
autofluorescence. 2D images at various depths of z-
axis from 0 to 10 lm are shown in Fig. 4. Orientation
of micrometer-sized emission tracks is closely depen-
dent of z-position. Each 1 micrometer change in depth
of the focal plane occur loss of orientation. This effect
may be related to the SEM images of the bagasse
sample in Fig. 1a, where oriented walls of the fiber are
located near its surface.
Lifetime measurements in combination with
microscopy techniques can be used to study biological
materials (Ulrich et al. 2004; Heskes et al. 2012).
Samples were investigated by fluorescence decay
measurements to identify lignin-rich regions. Fluores-
cence decay traces were recorded at a wavelength of
500 nm, as well as at 575 nm for samples with added
safranine, which corresponds to its emission maxi-
mum. Decay analyses were performed by FAST
software (Edinburgh Instruments) using multiexpo-
nential fitting without deconvolution. The fitting range
was chosen by considering the decay part of the time
dependent data according to optimal parameters.
Typical decay profiles of untreated and bleached
Fig. 4 Two-photon fluorescence microscope images of a whole
bagasse sample obtained at a focal plane of a 0 lm, b 5 lm and
c 10 lm. Scale bar 10 lm. The lateral color scale bars are
related to the fluorescence intensity
Cellulose
123
samples are illustrated in Fig. 3. The fluorescence
relaxation was fitted with a biexponential decay
function. The decay components, respective normal-
ized amplitudes and average values are presented in
Table 1. A fast decay component occurs in the range
of 0.4–1.4 ns, and a long-lived component takes more
than 2.0 ns to decay. Such biexponential decay
behavior with a short decay component of about
0.4 ns was first observed in the fluorescence emission
of Abies wood (Castellan and Davidson 1994).
Departure from single exponential decay behavior
is expected for a complex matrix like bagasse that
contains multiple intrinsic fluorophores such as aro-
matic compounds with phenolic and acid groups from
the lignin fraction (cinnamic residues), and traces of
endogenous biomolecules such as enzymes and
cofactors, chlorophyll, xanthophylls, coumarin and
flavonoid derivatives (Olmstead and Gray 1997;
Schwille et al. 1999; Albinsson et al. 1999; Billinton
and Knight 2001). Hafren and Oosterveld-Hut (2009)
studied wood fibers using fluorescence lifetime imag-
ing. Biexponential fitting at two emission regions of
436 and 480 nm resulted in wavelength-independent
decay times of about 0.7 and 4.3 ns. These values are
within the range of decay times observed for our
samples. For bagasse samples without added safra-
nine, the decay times were almost independent of
wavelength.
Analysis of decay parameters in this system is a
difficult task because of its complexity. Nevertheless,
some important issues were identified. In general, the
fluorescence decay of untreated and bleached samples
is nonexponential and occurs in\20 ns, as illustrated
in Fig. 3. The calculated average decay time increases
by about 68 % from fiber to BF, 47 % from whole
bagasse to BWB, and 41 % from pith to BP (see
Table 1). Samples stained with safranine show
slightly different decay behavior, as illustrated in
Fig. 5. First, unbleached samples like whole bagasse
show a third decay component with a lifetime of
4.8 ns. This component is ascribed to the decay of the
singlet excited state of safranine formed mainly
through energy transfer from the natural compounds
to the added dye. In addition, the fluorescence lifetime
of safranine in other solvents was also measured. In a
polyvinylpyrrolidone film, a single component with a
lifetime of about 4 ns was recorded, while the
fluorescence lifetime of safranine in propanol was
3 ns. Therefore, the observed increase of safranine
fluorescence lifetime in bagasse samples is a result of
absorption of the dye in lignin-rich regions. The
second difference is the moderate quenching of the
second decay component of the whole bagasse sample,
which is reduced from 1.9 to 1.3 ns. This result is
consistent with fluorescence quenching of excited
chromophores of the lignin fraction by energy transfer
to the adsorbed safranine. Fluorescence behavior is
closely linked to the chemical environment of the
cellulosic matrix (Castellan et al. 2007). Chemical
bleaching causes lignin components to be decomposed
and dispersed. The bleaching reaction also decreases
the amount of organic materials and intrinsic fluoro-
phores in the sample. Therefore, bleaching reduces
energy migration and fluorescence self-quenching in
Table 1 Decay times (si) and normalized amplitudes (ai) of micrometer-sized emission spots from cellulose samples isolated from
sugarcane bagasse obtained by multiexponential decay fitting
Sample s1 (ns) s2 (ns) s3 (ns) a1 a2 a3 hsi v2
Whole bagasse (500 nm) 0.4 1.9 0.43 0.57 1.7 1.15
Whole bagasse/safranine (500 nm) 0.8 2.8 0.71 0.29 2.0 1.20
Whole bagasse/safranine (575 nm) 0.4 1.3 4.8 0.73 0.23 0.04 2.0 1.05
BWB (500 nm) 0.9 3.1 0.58 0.42 2.5 1.03
BWB/safranine (500 nm) 0.8 3.3 0.56 0.44 2.7 1.13
BWB/safranine (575 nm) 1.1 2.8 0.44 0.56 2.2 1.00
Fiber (500 nm) 0.7 2.4 0.63 0.37 1.6 1.18
Pith (500 nm) 0.7 2.2 0.61 0.39 1.7 1.16
BF (500 nm) 0.9 3.4 0.60 0.40 2.7 1.12
BP(500 nm) 0.7 2.7 0.39 0.61 2.4 1.05
hsi = Amplitude-weighted average decay time
Cellulose
123
the samples. Self-quenching is mainly observed when
the lignin matrix is intact and its intrinsic fluorophores
are closely confined. The emission intensity of the
bleached samples is still strong because most of the
remaining chromophores are partially isolated or
dispersed in the cellulosic matrix, reducing excited-
state deactivation by self-quenching. These results are
in agreement with those obtained by Coletta et al.
(2013) using fluorescence lifetime imaging (FLIM) to
map the distribution of lignin in sugarcane bagasse.
They also obtained two components related to
fluorescence decay, one with the fast and another
with the slow decay time. The faster decay is
associated to dense lignin regions and becomes slower
after samples undergo pretreatment to remove lignin.
Emission spectra of the fiber samples were also
measured under the same conditions; the results are
depicted in Fig. 6. Untreated fiber exhibited high
intensity emission with a maximum at about 500 nm,
consistent with the emission spectra reported for wood
samples (Donaldson et al. 2010). When safranine was
added to the fiber sample, the emission was quenched
Fig. 5 Fluorescence intensity images and decay of each
indicated emission spot obtained by two-photon excitation at
800 nm of samples stained with safranine: a whole bagasse and
b BWB. Scale bar 10 lm. The lateral color scale bars are
related to the fluorescence intensity
Cellulose
123
and a new band appeared at about 575 nm corre-
sponding to the fluorescence of the added dye.
Safranine has negligible absorption at an excitation
wavelength of 405 nm, so dye emission may occur
after energy transfer from the intrinsic fluorophores to
safranine. The BF sample exhibited a similar emission
profile to that of the untreated fiber, but its intensity
was reduced by half. The reduction in intensity
confirms that chemical bleaching removed the lignin
fraction, so autofluorescence from the sample
decreased. However, the intensity is much higher than
would be expected from a sample containing a lignin
fraction of about 1 % after chemical bleaching. This
means that intrinsic fluorophores remained in some
regions of the sample, and these showed higher
emission efficiency than in the unbleached sample
because of matrix dispersion and less self-quenching.
Chemical treatment cleaves the lignin macrostructure
into smaller components, which then disperse over the
solid matrix, reducing self-quenching. For the BF
sample stained with safranine, the dye emission still
appears but at lower intensity, which agrees with
energy transfer occurring from the fluorophores
remaining in the sample to the added safranine dye.
The reference Avicel sample exhibited very weak
emission under the same conditions compared with
that from bagasse samples.
Conclusions
We used two-photon fluorescence microscopy to
characterize the autofluorescence from micro-regions
of sugarcane bagasse samples. Fluorescence images
show that fibril packages of bagasse sample partially
lose their longitudinal orientation after chemical
bleaching. Extraction of lignin allows the remaining
natural fluorophores to disperse in the sample, which
reduces self-quenching. The presence of highly emis-
sive spots after chemical bleaching indicates that
fluorescent lignin derivatives remain in some regions
of the lignocellulosic matrix. This result may indicate
the region where autocatalytic acid hydrolysis of
cellulose could start (Gehlen 2009, 2010).
Our results are able to provide information related
to the morphological properties and lignin distribu-
tion. In addition, it is possible to understand how these
parameters are affected by the bleaching process.
Therefore, this study provides support for future site-
specific morphological analyses of the effects of using
different pretreatments on cellulose hydrolysis. Con-
sequently, it acts in the field of second generation
bioethanol production.
Acknowledgments The authors thank the Conselho Nacional
de Desenvolvimento Cientıfico e Tecnologico and Coordenacao
Fig. 6 Fluorescence
spectra from (solid curve)
fiber, (long dashed curve)
fiber/safranine, (two dotted
dashed curve) BF, single
dotted dashed curve) BF/
safranine and (shorted
dashed curve) Avicel.
Samples were excited at
405 nm and spectral
intensity was recorded using
a linear CCD spectrometer
fiber coupled to the
binocular side port of the
microscope
Cellulose
123
de Aperfeicoamento de Pessoal de Nıvel Superior Brazilian
research funds. M.H.G. thanks Fundacao de Amparo a Pesquisa
do Estado de Sao Paulo for financial support that allowed a
fluorescence confocal microscope to be built. We thank
Professor Dr. Johan Hofkens and Dr. Kris P. F. Janssen for the
use of SIS software from the MDS Laboratory of the
Department of Chemistry of Katholieke Universiteit Leuven.
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