pubs.acs.org/journal/ascecg
Research Article
Enhancing Enzyme-Mediated Hydrolysis of Mechanical Pulps by
Deacetylation and Delignification
Jie Wu, Richard P. Chandra,* Kwang Ho Kim, Chang Soo Kim, Yunqiao Pu, Arthur J. Ragauskas,
and Jack Nicholas Saddler*
Cite This: ACS Sustainable Chem. Eng. 2020, 8, 5847−5855
Downloaded via UNIV OF TENNESSEE KNOXVILLE on April 24, 2020 at 09:10:02 (UTC).
See https://pubs.acs.org/sharingguidelines for options on how to legitimately share published articles.
ACCESS
Metrics & More
Read Online
Article Recommendations
sı Supporting Information
*
ABSTRACT: Alkaline induced deacetylation of the hemicellulose
combined with subsequent mechanical refining enhanced the
enzyme-mediated hydrolysis of pretreated corn stover. The
addition of either NaOH (80 °C) or mild KOH (25 °C) to
corn stover prior to mechanical refining led to greater than 80%
deacetylation with the NaOH treatment also solubilizing lowmolecular-weight lignin that was enriched in β-O-4 linkages with
more than 25% and 13% of the total and surface lignin removed,
respectively. The influence of deacetylation and delignification
were further enhanced when NaOH was supplemented with 3%
Na2SO3, resulting in 100% deacetylation, 34% delignification, and
a >20% increase in the hydrolysis yield of the substrate xylan. A
milder KOH treatment resulted in the retention of more than 95%
of the lignin within the cellulose rich, water-insoluble fraction with no apparent change in the surface lignin. However, both methods
resulted in enhanced xylan hydrolysis when treated with xylanases, suggesting that deacetylation had enhanced accessibility to the
xylan present in the pretreated of corn stover. It was apparent that cellulose accessibility was also enhanced by partial delignification,
as NaOH treatment resulted in a 65% and 43% increase in the Water Retention Value and Directed Orange dye adsorption,
respectively.
KEYWORDS: Deacetylation, Delignification, Enzyme-mediated hydrolysis, Increased enzyme accessibility
high yield pulps that are primarily used to produce newsprint.9
However, as the newsprint market has declined, primarily due
to the growth of digital media,9 mechanical pulping has been
more recently assessed as a potential front-end/pretreatment
step for enzyme mediated bioconversion processes.8,10−12 The
earlier work showed that although mechanical refining did
increase the external surface area of the fibers, both the lignin
and hemicellulose retention properties of mechanical pulping
appeared to limit enzyme accessibility to the cellulose.6,13
Other recent work has shown that mild-alkali treatment (4.8%
NaOH) resulted in the deacetylation of mechanically refined
corn stover hemicellulose,14 enhancing enzyme accessibility to
the cellulose and xylan while decreasing potential inhibitors
due to the prior removal of most of the liberated acetic
acid.13,15
INTRODUCTION
One of the main goals of the pretreatment step in a biomassto-sugars process is to recover as much of the cellulose and
hemicellulose as possible while increasing the accessibility of
these carbohydrates to enzymes.1 Although pretreatments
using dilute acid and steam have been shown to solubilize the
hemicellulose component, consequently increasing accessibility
to the cellulose component,2,3 these methods typically produce
inhibitors such as acetic acid, phenols, furfural, and
hydroxymethylfurfural (HMF) that result from the degradation
of hemicellulose and lignin.4 Acidic pretreatments have also
been shown to condense the lignin, decreasing substrate
swelling and enzyme accessibility to the cellulose component
and contributing to the nonproductive binding of cellulases to
the lignin.5,6 The condensation of lignin also decreases its
potential utility as a value-added coproduct.
Similar to the work of other groups, we assessed alkaline
pretreatments such as sodium hydroxide, alkaline-oxygen,
sulfite and ammonia freeze expansion (AFEX) as one way of
retaining all of the biomass components in a “single-pot”, while
modifying the lignin and/or hemicellulose to enhance enzyme
accessibility to the cellulose.7,8 As detailed elsewhere,
mechanical pulping is a commercial process that results in
■
© 2020 American Chemical Society
Received: December 3, 2019
Revised: February 26, 2020
Published: March 24, 2020
5847
https://dx.doi.org/10.1021/acssuschemeng.9b07226
ACS Sustainable Chem. Eng. 2020, 8, 5847−5855
ACS Sustainable Chemistry & Engineering
pubs.acs.org/journal/ascecg
Along with deacetylating the hemicellulose,16 NaOH
addition has also been shown to readily ionize phenols and
dissolve low molecular weight lignins.17−19 As the lignin in
agricultural residues is also rich in hydrophilic coumaric and
ferulic acid subunits, it is likely to be more susceptible to
dissolution after NaOH treatment at mild conditions.20,21
Earlier work has shown that close to 20% of the lignin could be
removed after treatment at these conditions.14 As mentioned
earlier, lignin impedes hydrolysis by both restricting substrate
swelling and nonproductive binding to enzymes.6,22,23
In the work reported here both lignin removal and
modification as well as hemicellulose deacetylation influenced
the effectiveness of enzyme mediated hydrolysis of cellulose.
As previous work had shown that sulfite addition under
alkaline conditions improved hydrolysis by enhancing fiber
swelling and reducing nonproductive lignin binding,5,6 its
addition was shown to increase lignin removal and hemicellulose deacetylation, enhancing both xylan and cellulose
hydrolysis.
■
Research Article
nm) and an HPLC (ICS-500) equipped with an Aminex HPX-87H
column (Bio-Rad, Hercules, CA).
Acid Group Titration. The conductometric titration of acid
groups was carried out using a modified version of the method
developed by Katz et al.26 Briefly, 0.15 g (OD basis) of the substrate
was soaked with 15 mL of 0.1 N HCl overnight, followed by washing
and filtration using 250 mL DI water in a Buchner funnel. The washed
substrate was then transferred to a plastic beaker and resuspended in
50 mL of 0.001 M NaCl solution. After the addition of 200 μL of 0.05
N HCl, 0.05 M NaOH was added to the mixture, at increments of 20
uL, to titrate the acid groups.
Simons’ Stain. The high-molecular-weight fraction of Direct
Orange 15 (DO) dye was isolated and used for the Simon’ stain
method according to Chandra et al.27 Briefly, a set of 10 mg (OD
basis) of substrates were soaked with deionized water and PBS buffer
in 2 mL screw cap tube (Eppendorf) overnight prior to the incubation
with DO dye in the shaking incubator at 60 °C and speed of 180 rpm
overnight. After centrifugation, the absorbance of the supernatant at
450 nm was measured using a spectrophotometer.
Water Retention Value (WRV). The WRV was measured (in
triplicate) using TAPPI Useful Method-256. Briefly, around 0.5 g
(OD basis) of the substrate was soaked in 50 mL of DI water
overnight and filtered through a 200-mesh screen in the WRV unit.
The pulp pad after filtration was centrifuged at 900 RCF for 30 min
and subject to oven drying.
The WRV was calculated using the equation: WRV = (Wet mass −
Dry mass)/Dry mass, where the wet mass is the weight of the wet
sample after the centrifugation and the dry mass is the weight of the
dried sample.
X-ray Photoelectron Spectroscopy (XPS). The substrate was
disintegrated and filtered in a Buchner funnel to form a substrate
sheet (80 g/m2), which was then dried and pressed at 40 psig for 5
min. The XPS measurements were conducted using a Leybold Max
200 X-ray photoelectron spectrometer (Cologne, Germany) with a
monochromated Al Ka X-ray source. The detector position was at an
angle of 90 relatives to the sample surface. The theoretical surface
lignin coverage was calculated from the O/C ratios according to Laine
et al.28 using the following equation: Surface lignin coverage Φ lignin=
(O/C (Sample) − O/C (cellulose))/ (O/C (lignin) − O/C (cellulose)), where
O/C (sample) is the O/C ratio of the analyzed sample, and O/C (cellulose)
and O/C (lignin) are the theoretical O/C ratios of pure cellulose (0.83)
and lignin (0.33).
Lignin Isolation from the Deacetylation Liquor. The
precipitation of lignin from the deacetylation liquor was carried out
by lowering the pH of the deacetylation liquor to pH 2. The
precipitated lignin was collected through centrifugation, washed with
deionized water, and freeze-dried.
Lignin Acetylation and Gel Permeation Chromatography
(GPC). Lignin samples were acetylated to allow dissolution in
tetrahydrofuran (THF) prior to GPC analysis. In brief, 50 mg of
lignin was mixed with 3 mL each of pyridine and acetic anhydride
(1:1) in round-bottom flasks. The mixture was stirred at 70 °C for 1
and 72 h at room temperature. Ethanol (30 mL) was added to the
mixture, and the mixture was concentrated in a rotating evaporator
under reduced pressure. This procedure was repeated 3 times to allow
for complete removal of the pyridine and acetic anhydride. Acetylated
lignin was dissolved in chloroform, washed twice with DI water in a
separatory funnel, and dried over sodium sulfate. The lignin was
precipitated in diethyl ether and dried in a 40 °C vacuum oven for 24
h. The acetylated lignin sample was then dissolved in anhydrous THF
at a concentration of 5 mg/mL and stored at room temperature for 48
h prior to filtration via 0.45 μm PTFE syringe filters and GPA
measurement.
GPC measurements were conducted using Agilent 1100 GPC
equipment (USA), equipped with three different columns including
Styragel HR4 (5−600 kDa), HR3 (0.5−30 kDa) and HR1 (0.1−5
kDa). The eluting solvent, THF, was used as the mobile phase, at a
flow rate of 0.7 mL/min. In brief, the system injected 100 μL of each
lignin solution and separated them into different molecular weights.
The samples are then analyzed using a Wyatt Optilab T-Rex refractive
MATERIALS AND METHODS
Biomass and Chemicals. Corn stover was provided by
Novozymes (Davis, California). Sodium hydroxide, potassium
hydroxide, and sodium sulfite were purchased from VWR International.
Deacetylation Treatments. NaOH-based deacetylation of corn
stover was conducted according to Chen et al.19 Briefly, 50 g of ovendried (OD) corn stover was impregnated with 4.8% (w/w) NaOH
(12:1 liquid/wood ratio, 0.1M) in an 80 °C water bath for 3 h. For
Na2SO3/NaOH deacetylation, an additional 3% (w/w) of Na2SO3
was added to the NaOH solution prior to the impregnation, with the
4.8% NaOH replaced by 3% Na2SO3 for the sulfite control group. The
KOH-based deacetylation of corn stover used the method described
by Jiang and Xu.24 Briefly, 50 g (OD basis) of corn stover was
impregnated with 7.5% (20:1 liquid/wood ratio, 0.07M) in a 25 °C
water bath for 24 h. The chemically/water treated corn stover samples
were subsequently refined at room temperature using a commercial
juicer (super angel juicer model 8500) and a total volume of 10 L of
water, followed by PFI milling for 2000 revolutions, according to
TAPPI standard T-248 method. It was anticipated that the fiber
separation and fibrillation resulting from sequential juicer and PFI
milling treatment effectively mimicked industrial mechanical pulping
at a lab scale.
Enzymatic Hydrolysis. The protein content of the cellulase
enzyme mixture (Cellic CTec 3) and the xylanase (HTec) were
measured by the ninhydrin assay, as described by Mok et al.25 The
cellulase enzyme mixture was used to hydrolyze the corn stover
substrates whereas the xylanase was primarily used to assess the
accessibility of the xylan component. Enzymatic hydrolysis of corn
stover substrates at 2% solid loading was conducted in 2 mL screwcap
tubes (Eppendorf) containing acetate buffer (50 mM, pH 5.0) and
Cellic CTec 3. The mixture was placed in a rotating incubator at 50
°C for 48 h.
Chemical Composition Analysis. The chemical compositions of
the corn stover and isolated lignin were assessed using the TAPPI
standard T-22 om-88 method (in triplicate). Briefly, 0.2 g of
extractive-free substrate was Wiley milled and mixed prior to being
stirred with 3 mL of 72% H2SO4 for 2 h. The mixture was diluted with
112 mL of deionized (DI) water and autoclaved at 121 °C for 1 h.
The acid-insoluble lignin (AIL) was collected and measured using a
30 mL fritted glass crucible. The acid-soluble lignin (ASL) was
analyzed by determining the absorbance at 205 nm. The carbohydrate
components of the acid-soluble fraction were measured using a
Dionex (Sunnyvale, CA) HPLC (ICS-3000). The acetyl content was
determined as the acetic acid present in the acid-soluble fraction
according to Jiang and Xu,24 using a UV detector (wavelength of 280
5848
https://dx.doi.org/10.1021/acssuschemeng.9b07226
ACS Sustainable Chem. Eng. 2020, 8, 5847−5855
ACS Sustainable Chemistry & Engineering
pubs.acs.org/journal/ascecg
Research Article
Table 1. Chemical Composition, Sugar Recovery, and Lignin/Acetyl Removal of the Various Mechanically Pulped Corn Stover
Samples
Treatments
Starting corn stover
25 °C 24 h water
control
25 °C 24 h KOH
Deacetylation
80 °C 3 h water
control
80 °C 3 h NaOH
deacetylation
Cellulose
Content (%)
Lignin
Content (%)
Xylan
Content
(%)
Acetyl
Content
(%)
Pretreatment
yield (%)
Cellulose
Recovery (%)
Xylan
Recovery
(%)
lignin
Removal
(%)
Acetyl
Removal
(%)
42.3 ± 2.7
43.9 ± 0.4
19 0.3 ± 0.2
20.1 ± 1.0
21.8 ± 1.0
19.8 ± 0.5
3.1 ± 0
2.1 ± 0
N/A
95.0
N/A
98.6
N/A
86.0
N/A
1.2
N/A
32.0
48.6 ± 0.7
20 ± 0.8
23 ± 0.7
0.6 ± 0
93.4
107.3
97.2
5.9
81.0
42 ± 2.9
22 ± 0.2
21 ± 1.5
2.2 ± 0
78.0
76.4
73.1
12.8
29.0
53 ± 3.7
17.7 ± 0.5
24.6 ± 1.0
0.6 ± 0
81.2
100.8
91.6
25.6
80.0
index detector (dRI, USA), 785 nm at 35 °C. The data was collected/
analyzed by Wyatt ASTRA 6.0 (USA) and calibrated with polystyrene
standards.
Two-Dimensional Heteronuclear Single-Quantum Correlation NMR (2D HSQC NMR). The lignin was dissolved in DMSO-d6
prior to 2D 1H-13C HSQC NMR analysis, using a Bruker Avance III
400-MHz spectrometer. The method is described in detail by Yao et
al.29 and Liu et al.30 After the acquisition of the HSQC spectra, the
relative abundance of the lignin compositional subunits and interunit
linkages was assessed using volume integration of cross peak contours.
Elemental Analysis. The elemental analysis of the corn stover
substrates (C, H, N, and S) was assessed using a Thermo Flash 2000
Elemental Analyzer. Substrates were oven-dried, Wiley milled, and
stored in the 1.5 mL centrifuge tube prior to analysis.
1). In contrast, the room temperature control retained the
majority of the carbohydrates and lignin within the waterinsoluble fraction (Table 1). It is probable that the hot water
(80 °C) control was acting as a milder version of “autohydrolysis”, where the initial removal of acetyl groups was
facilitated, consequently releasing protons43,44 which resulted
in mild acidolysis and the dissolution of a small amount of
lignin.35
It was apparent that the addition of either the NaOH or
KOH enhanced deacetylation, as 80% of the acetyl groups
were removed from the corn stover regardless of whether the
reaction was performed at 80 °C or at room temperature
(Table 1). However, the NaOH treatment at 80 °C for 3 h
resulted in the removal of more lignin (>25%) as compared to
the KOH 24-h treatment at room temperature (Table 1). As
the two alkaline treatments resulted in similar amounts of
deacetylation, but differed in the extent of lignin removal, these
treatments were next compared to try to better elucidate the
relative influence of deacetylation and delignification on the
enzymatic hydrolysis of pretreated corn stover.
As previous work has shown that the addition of accessory
enzymes such as xylanases enhanced the hydrolysis of the
cellulose component of pretreated corn stover,45 it was
anticipated that these xylan rich substrates could provide a
good indication of the influence of deacetylation on the
hydrolysis of both of the cellulose and the xylan components.46
As indicated in Figure 1, deacetylation significantly enhanced
the hydrolysis of both cellulose and hemicellulose. However, it
was likely that the observed 25% delignification resulting from
NaOH treatment at 80 °C also helped increase cellulose and
RESULTS AND DISCUSSION
Previous work has shown that deacetylation enhances enzymemediated hydrolysis of biomass16,19,31 with the alkali
concentration, residence time, and temperature all influencing
the extent of deacetylation. At room temperature, longer
residence times (24 h) and higher alkaline concentrations
(0.1−0.2 M) have been used to deacetylate agricultural and
hardwood substrates,16 while at higher temperatures (70−100
°C), lower alkali charges(<0.01 M) and shorter residence
times have been successfully used.32 As the temperature is
increased, up to 20% of the lignin can be removed,19 likely due
to the hydrolysis of LCC ester linkages33and the ionization of
the phenolic and carboxylic functionalities in lower molecular
weight lignin fragments. This process has some similarity to
the alkaline extraction step employed during pulp bleaching.34−36 As mentioned earlier, lignin has been shown to
impede cellulose hydrolysis by restricting substrate swelling
and nonproductively binding cellulase enzymes.23,37,38 As
previous work had shown that the removal of even a small
amount lignin from the pretreated biomass could significantly
enhance enzymatic hydrolysis as well as decrease the
nonproductive binding of cellulases,39,40 the primary goal of
this work was to better elucidate the relative contribution of
deacetylation and delignification to enhancing the enzymatic
hydrolysis of corn stover.
As NaOH-based deacetylation had been successfully used by
Chen and others,11,19,41,42 we first wanted to compare this
method to a milder, KOH treatment at room temperature that
had previously been shown to selectively remove acetyl
groups.16,24 Controls, in the absence of added alkali, were
carried out at both 80 °C and at room temperature. Likely due
to the labile nature of the ester linkages within the
hemicelluloses, the control at 80 °C resulted in the removal
of about 30% of the acetyl groups, the solubilization of around
25% of the carbohydrates, and about 10% of the lignin (Table
■
Figure 1. Enzymatic hydrolysis of mechanically pulped corn stover.
Hydrolysis was conducted at 2% (w/v) solids and enzyme loading of
20 mg g−1 cellulose in a rotating incubator at 50 °C for 48 h.
5849
https://dx.doi.org/10.1021/acssuschemeng.9b07226
ACS Sustainable Chem. Eng. 2020, 8, 5847−5855
ACS Sustainable Chemistry & Engineering
pubs.acs.org/journal/ascecg
Research Article
overall lignin could reduce the nonproductive binding of
enzymes to the substrate,40 the relative surface lignin of the
deacetylated and untreated corn stover biomass was measured
using X-ray Photoelectron Spectroscopy (XPS). As detailed
previously, the XPS method measures the oxygen to carbon
ratio28,48 of the substrate surface, at a depth of 5−10 nm, to
estimate the relative amount of lignin that is present, with an
increase in surface lignin indicated by an increase in measured
surface carbon and a reduction in oxygen.49 It was apparent
that compared to the negligible effect of KOH treatment at
room temperature, the NaOH treatment at 80 °C was able to
remove more than 12% of the surface lignin (Table 2). This
xylan hydrolysis, suggesting that both deacetylation and
delignification contributed to the observed increase in
hydrolysis.
Although both the mild KOH and NaOH treatments
resulted in about the same amount of deacetylation (Table 1),
it was apparent that the xylan contained in the substrate
resulting from the KOH treatment at room temperature was
less susceptible to enzymatic hydrolysis than the xylan
component of the NaOH-treated substrate (Figure 1). This
result suggested that in addition to deacetylation, partial
delignification had also enhanced xylan accessibility; we next
added xylanases (Novozymes HTec) to each of the pretreated
substrates to see if enzyme accessibility had in fact increased.
Medium-to-relatively high-loadings of xylanase (25 and 50 mg
xylanase/g of cellulose) were used to ensure that the use of low
enzyme concentrations did not influence the results. The xylan
in the deacetylated corn stover substrates appeared to be more
accessible to the xylanases, particularly within the first 3 h
(Figure 2), although the xylan in all of the substrates was
Table 2. Substrate Swelling, Accessibility, and Enzymatic
Hydrolysis of Mechanically Pulped Corn Stover
Treatment
Mechanical
refining
25 °C 24 h water
control
25 °C 24 h
KOH
deacetylation
80 °C 3 h water
control
80 °C 3 h
NaOH
deacetylation
Surface
lignin
(%)
Water
Retention
Water
DO
adsorption
(mg/g)
Total acid
groups
(mmol/kg)
82.6
2.0 ± 0.0
58.3
113 ± 14
2.3 ± 0.0
54.3
100 ± 7
2.6 ± 0.1
76.3
157 ± 10
2.8 ± 0.0
75.0
106 ± 17
3.3 ± 0.2
83.3
166 ± 10
85.1
71.9
suggested that the removal of the lignin, particularly at the
substrate surface, resulted in the increased overall enhanced
enzyme accessibility and hydrolysis of the NaOH treated
substrates.
In past work, the water retention value (WRV) has been
used to assess a pulp or pretreated substrate’s accessibility to
water and this value is typically used to provide an estimate of
fiber swelling.50,51 In contrast to the WRV, the Simon’s
staining technique utilizes a Direct Orange (DO) dye that has
a similar size to the predominant cellulase enzyme,
cellobiohydrolase, and has been successfully used to estimate
the enzyme accessibility of a substrate.27,52−54 When the five
substrates were compared (Table 2), the NaOH treatment
resulted in the largest increase in cellulose accessibility when
compared to the mechanical pulp control (65% increase in
WRV and 43% increase in DO adsorption). This enhanced
accessibility was likely due to the removal of much of the
surface lignin as well as the embedded lignin which facilitated
substrate swelling (Table 2). Although the KOH and water
treatments at 80 °C also enhanced substrate swelling and
cellulose accessibility, it was to a considerably lesser extent
(Table 2). Although the removal of around 30% of the xylan as
well as 13% of the lignin after hot water (80 °C) treatment
likely resulted in enhanced swelling and cellulose accessibility,
KOH treatment did not cause a significant change in the
chemical composition of the substrate other than deacetylating
the xylan (Table 1). It should be noted that the KOH
treatment of corn stover gave results that were similar to those
previously observed after Ammonia Freeze Expansion treatment (AFEX). This pretreatment has been shown to
selectively deacetylate the xylan present in agricultural biomass
such as corn stover, consequently increasing cellulose
accessibility while resulting in only limited changes to the
Figure 2. Xylan hydrolysis of deacetylated and control samples of
mechanically pulped corn stover at high enzyme loadings and short
incubation times. Hydrolysis was conducted at 2% solid at 50 °C for 3
and 24 h.
partially hydrolyzed after 24 h. The slightly higher hydrolysis
yields of the xylan present in the NaOH treated substrates after
hydrolysis with the CTec 3 cellulase mixture was likely due to
the synergistic action of the cellulases hydrolyzing the cellulose
which consequently exposed the xylan previously “buried”
within the fiber structure to the xylanases.45 Although the 3-h
water treatment at 80 °C increased the CTec 3 induced
hydrolysis of both the cellulose and xylan (Figure 1), much
lower hydrolysis yields were obtained when xylanase alone
(HTec) was added (Figure 2). It is likely that the hot water
treatment resulted in the removal of the more easily accessible
xylan, consequently exposing more of the cellulose that was
more readily hydrolyzed by the CTec 3 mixture (Figure 1).
Although the NaOH and KOH deacetylation treatments
appeared to enhance xylan accessibility to similar extents, it
was not clear if the major benefit of the treatments was due to
deacetylation rather than delignification. In addition to
enhancing xylan hydrolysis, it was apparent that the NaOH
treatment resulted in the removal of 25% of the lignin which
also likely contributed to the observed increase in cellulose
hydrolysis. Previous work has shown that just like the overall
total lignin content, the surface lignin in particular plays a
significant role in influencing enzymatic hydrolysis.47 As other
workers had shown that the removal of as little as 3% of the
5850
https://dx.doi.org/10.1021/acssuschemeng.9b07226
ACS Sustainable Chem. Eng. 2020, 8, 5847−5855
ACS Sustainable Chemistry & Engineering
pubs.acs.org/journal/ascecg
Research Article
Table 3. Molecular Weight and Structure of Isolated Lignin from the Deacetylation Liquor and EMAL lignin Derived from
Corn Stover, Analyzed by Gel Permeation Chromatography (GPC) and HSQC NMR
Lignin structurea
Interlinkages (%)
Lignin subunits (%)
Weight-Average Molecular Weight (kDa)
β-O-4
α-O-4/ β −5
β−β
Cinnamyl alcohol
S
G
H
p-CAb
Ferulateb
S/G ratio
8.1
40.1
5.2
0.9
2.3
43.3
44.4
12.3
24.7
9.5
0.98
a
b
Calculated based on the total S+G+H aromatic ring. Results expressed per 100 Ar. p-Coumarate (p-CA) and Ferulate levels are expressed as a
fraction of S + G + H.
Figure 3. HSQC Spectrum of lignin isolated from the deacetylation liquor.
chemical composition of the substrates.55,56 Thus, as suggested
previously, it is likely that selective deacetylation, through the
cleavage of ester bonds between the xylan backbone and the
pendant acetyl groups, increased enzyme accessibility to the
xylan and the cellulose.13,15,16 As there are also a significant
number of ester bonds that link uronic acids and cinnamic
acids to corn stover xylan,57−60 it is also likely that the cleavage
of ester bonds during the alkaline treatments exposed more of
the weaker acid groups.61 Thus, it is probable that this
contributed to the observed increase in substrate swelling, as
described previously.62 In addition, it was also possible that the
cleavage of ester bonds contributed to enhancing the
accessibility of the xylan backbone to xylanases. When the
strong and weak bulk acid groups in the various substrate were
assessed using conductometric titration (Table 2), the alkaline
treatments were shown to result in a 50% increase in overall
total acid groups. This suggested that both the alkaline and hot
water treatments enhanced swelling and cellulose accessibility
through a combination of lignin/hemicellulose removal as well
as through the enrichment of acid groups within the substrate.
Due to the mild nature of the NaOH treatment at 80 °C, it
was anticipated that the solubilized lignin would be of a low
molecular weight. When alkaline pulping is used to produce
paper making pulps, it is typically far more aggressive than the
deacetylation treatments used here and results in the cleavage
of ether bonds and the formation on new phenolic end
groups.63,64 Therefore, the milder alkaline treatment that had
been used for deacetylation was expected to solubilize lignin
that retained its native ether and carbon−carbon bond
structure to a greater extent than that which occurred after
either pulping or acid pretreatments.65,66 When the molecular
weight and chemical characteristics of the lignin present in the
deacetylation liquor were compared to those of enzyme mild
acidolysis lignin (EMAL) isolated from the original corn stover
biomass (Song et al.67), the average molecular weight of the
deacetylation liquor lignin was much lower than that of the
5851
https://dx.doi.org/10.1021/acssuschemeng.9b07226
ACS Sustainable Chem. Eng. 2020, 8, 5847−5855
ACS Sustainable Chemistry & Engineering
pubs.acs.org/journal/ascecg
Research Article
Table 4. Recovery of Biomass Chemical Components and Substrate Characteristics after the Treatments of NaOH/Na2SO3
and Na2SO3 Combined with Mechanical Refining to Corn Stover
Samples
80 °C 3 h NaOH/
Na2SO3
deacetylation
80 °C 3 h 3%
Na2SO3 control
Total Acid
groups
(mmol/kg)
Water
Retention
Water
DO
adsorption
(mg/g)
Pretreatment
yield (%)
Cellulose
recovery
(%)
Xylan
recovery
(%)
lignin
removal
(%)
Acetyl
Removal
(%)
Cellulose
hydrolysis
(%)a
Xylan
hydrolysis
(%)a
163 ± 10
2.8 ± 0.1
83
81.4
102.1
92.9
34.3
100.0
71 ± 1
78 ± 2
147 ± 13
2.3 ± 0.1
62
89.3
98.0
93.1
4.5
30.0
41 ± 1
40 ± 1
a
Enzymatic hydrolysis was conducted at 2% solid and protein loading of 20 mg g−1 cellulose at 50 °C for 48 h.
been added at a loading of 4.8% during the deacetylation
reactions, it is possible that the NaOH treatment at 80 °C was
able to simultaneous deacetylate the hemicellulose and
sulfonate the corn stover lignin, further enhancing subsequent
hydrolysis.
It was apparent that the addition of 3% Na2SO3 during the
deacetylation reaction further enhanced the removal of lignin
and acetyl groups from corn stover to 34% and 100%,
respectively, while retaining most of the carbohydrate (Table
4). Although lignin removal was enhanced by the addition of
sulfite during the deacetylation reaction, enhanced sulfonation
of the residual lignin was not detected by conductometric
titration (Table 4). Similarly, elemental analysis of the NaOH/
Na2SO3 treated sample also did not show any sulfur
incorporation onto the corn stover during treatment (Table
S2). However, it is likely that the addition of sulfonic acid
groups facilitated the dissolution of a greater amount of the
low molecular weight lignin as the lignin became more
hydrophilic and ionizable. It was also likely that the increased
dissolution of lignin exposed a greater amount of xylan, which
could be further deacetylated by the added hydroxide ions.
Consequently, the addition of Na2SO3 to the NaOH during
the deacetylation process also resulted in a >20% enhancement
in the hydrolysis of the xylan (Figure 1, Table 4). In contrast,
the addition of Na2SO3 to the corn stover in the absence of
alkali did not result in any further increase in the solubilization
of acetyl groups, lignin, or carbohydrates (Table 4), suggesting
the synergistic action of alkali with the sulfite had enhanced
both lignin removal and xylan deacetylation.
EMAL lignin (Table 3). As anticipated, the lower temperature
alkaline treatment had removed the smaller fragments of lignin
that were more readily ionized under alkaline conditions.
When Heteronuclear Single-Quantum Correlation NMR
(HSQC-NMR) was used to analyze the low-molecular-weight
lignin (Figure 3), it was apparent that this solubilized lignin
retained up to 40% of its native β-O-4 bonds (Table 3). This
was comparable to the amount β-O-4 linkages detected in corn
stover milled wood lignin, indicating that the solubilized lignin
retained much of its native structure.20 This, in combination
with other features from lignin such as <1% of β−β bonds and
an syringyl/guaiacyl (S/G) ratio that was close to the original
corn stover lignin (Table 3),68 strongly suggested that this
lignin fraction underwent limited changes during solubilization.
This was consistent with recent work which showed that
lignins isolated at lower temperature by methods such as DES
and p-TsOH hydrotrope were structurally similar to the
original biomass lignin.69 The HSQC analysis also indicated
the presence of p-coumarate and ferulic acids in corn stover
lignin, as reported previously,20,70 supporting the notion that
carboxylic groups, which are readily ionized at pH > 5,
facilitated the dissolution of this low molecular lignin fraction.
The HSQC-NMR spectrum also indicated that carbohydrates
were present in the lignin sample (Figure 3) with subsequent
analysis indicating that xylan had been solubilized with the
lignin during alkaline treatment (Table S1). It is likely that the
xylan was linked to lignin through lignin-carbohydrate
complexes via the ester and ether bonds that are prevalent in
corn stover biomass.20,33,59,60 The attractive properties of this
lignin fraction, such as its low molecular weight, high
percentage of native linkages, and semihydrophilic properties,
make it a possible source of aromatics for the production of
renewable chemicals via both chemical71,72 and biological
pathways.73,74
As it was likely that the removal of low molecular weight
lignin, especially from the surface of corn stover during the
mild NaOH treatment at 80 °C, played a significant role in
enhancing cellulose accessibility to enzymes, we wanted to
further investigate how much deacetylation had contributed to
this enhancement. Previous work had shown that an alkaline
environment was beneficial to the incorporation of sulfonic
acids to lignin by deprotonating phenolic lignin moieties that
were susceptible to nucleophilic attack by sulfite anions.5,35 In
related work, sulfonated lignin has been shown to be less
restrictive to substrate swelling and also has a lower tendency
to bind enzymes due to its increased hydrophilicity.22,75
Although several studies have looked at sulfonation at
temperatures above 100 °C, recent work by Zhong et al.76
showed that 106 mmol/kg of sulfonic acid groups could be
incorporated into softwood lignin at a temperature of 70 °C
using 2% alkali. In the work reported here, as the NaOH had
CONCLUSIONS
Previous work had suggested that during alkaline pretreatment
of agricultural biomass, deacetylation of the hemicellulose was
the predominant mechanism which enhanced enzymemediated cellulose hydrolysis. However, alkaline mediated
deacetylation also resulted in partial delignification, particularly
at the substrate surface. It was apparent that lignin removal also
enhanced enzyme accessibility to the cellulose, resulting in
increased cellulose hydrolysis. The delignification and
deacetylation mechanisms were further enhanced by supplementing the alkaline solution with sodium sulfite. It was likely
that the sulfonation reaction facilitated lignin removal, which in
turn exposed more of the xylan to xylanases.
■
■
ASSOCIATED CONTENT
sı Supporting Information
*
The Supporting Information is available free of charge at
https://pubs.acs.org/doi/10.1021/acssuschemeng.9b07226.
Chemical composition of the precipitate from the
deacetylation liquor and elemental analysis of mechanically pulped corn stover (PDF)
5852
https://dx.doi.org/10.1021/acssuschemeng.9b07226
ACS Sustainable Chem. Eng. 2020, 8, 5847−5855
ACS Sustainable Chemistry & Engineering
■
pubs.acs.org/journal/ascecg
Research Article
not necessarily state or reflect those of the United States
Government or any agency thereof. Neither the United States
Government nor any agency thereof, nor any of their
employees, makes any warranty, expressed or implied, or
assumes any legal liability or responsibility for the accuracy,
completeness, or usefulness of any information, apparatus,
product, or process disclosed, or represents that its use would
not infringe privately owned rights.
AUTHOR INFORMATION
Corresponding Authors
Richard P. Chandra − Forest Products Biotechnology/Bioenergy
Group, Department of Wood Science, Faculty of Forestry,
University of British Columbia, Vancouver, BC V6T 1Z4,
Canada; orcid.org/0000-0003-1904-0750;
Email: richardchandra77@gmail.com
Jack Nicholas Saddler − Forest Products Biotechnology/
Bioenergy Group, Department of Wood Science, Faculty of
Forestry, University of British Columbia, Vancouver, BC V6T
1Z4, Canada; orcid.org/0000-0002-8689-3967;
Email: jack.saddler@ubc.ca
■
REFERENCES
(1) Chandra, R. P.; Bura, R.; Mabee, W. E.; Berlin, A.; Pan, X.;
Saddler, J. N. Substrate Pretreatment: The Key to Effective Enzymatic
Hydrolysis of Lignocellulosics? Adv. Biochem. Eng. Biotechnol. 2007,
108, 67−93.
(2) Linde, M.; Jakobsson, E. L.; Galbe, M.; Zacchi, G. Steam
Pretreatment of Dilute H2SO4-Impregnated Wheat Straw and SSF
with Low Yeast and Enzyme Loadings for Bioethanol Production.
Biomass Bioenergy 2008, 32, 326.
(3) Saha, B. C.; Iten, L. B.; Cotta, M. A.; Wu, Y. V. Dilute Acid
Pretreatment, Enzymatic Saccharification and Fermentation of Wheat
Straw to Ethanol. Process Biochem. 2005, 40, 3693.
(4) Palmqvist, E.; Hahn-Hägerdal, B.; Galbe, M.; Zacchi, G. The
Effect of Water-Soluble Inhibitors from Steam-Pretreated Willow on
Enzymatic Hydrolysis and Ethanol Fermentation. Enzyme Microb.
Technol. 1996, 19, 470.
(5) Chandra, R. P.; Chu, Q. L.; Hu, J.; Zhong, N.; Lin, M.; Lee, J. S.;
Saddler, J. The Influence of Lignin on Steam Pretreatment and
Mechanical Pulping of Poplar to Achieve High Sugar Recovery and
Ease of Enzymatic Hydrolysis. Bioresour. Technol. 2016, 199, 135−
141.
(6) Kumar, L.; Arantes, V.; Chandra, R.; Saddler, J. The Lignin
Present in Steam Pretreated Softwood Binds Enzymes and Limits
Cellulose Accessibility. Bioresour. Technol. 2012, 103 (1), 201−208.
(7) Chu, Q.; Chandra, R. P.; Kim, C. S.; Saddler, J. N. Alkali-Oxygen
Impregnation Prior to Steam Pretreating Poplar Wood Chips
Enhances Selective Lignin Modification and Removal While Maximizing Carbohydrate Recovery, Cellulose Accessibility, and Enzymatic Hydrolysis. ACS Sustainable Chem. Eng. 2017, 5 (5), 4011−
4017.
(8) Wu, J.; Chandra, R.; Saddler, J. Alkali-Oxygen Treatment Prior
to the Mechanical Pulping of Hardwood Enhances Enzymatic
Hydrolysis and Carbohydrate Recovery through Selective Lignin
Modification. Sustain. Energy Fuels 2019, 3, 227.
(9) Unece; Fao. The North American Forest Sector Outlook Study.
Geneva Timber For. Study 2006, 65.
(10) Zhu, J. Y.; Pan, X. J.; Wang, G. S.; Gleisner, R. Sulfite
Pretreatment (SPORL) for Robust Enzymatic Saccharification of
Spruce and Red Pine. Bioresour. Technol. 2009, 100, 2411.
(11) Chen, X.; Shekiro, J.; Pschorn, T.; Sabourin, M.; Tao, L.;
Elander, R.; Park, S.; Jennings, E.; Nelson, R.; Trass, O.; et al. A
Highly Efficient Dilute Alkali Deacetylation and Mechanical (Disc)
Refining Process for the Conversion of Renewable Biomass to Lower
Cost Sugars. Biotechnol. Biofuels 2014, 7, 98.
(12) Jones, B. W.; Venditti, R.; Park, S.; Jameel, H.; Koo, B.
Enhancement in Enzymatic Hydrolysis by Mechanical Refining for
Pretreated Hardwood Lignocellulosics. Bioresour. Technol. 2013, 147,
353.
(13) Selig, M. J.; Adney, W. S.; Himmel, M. E.; Decker, S. R. The
Impact of Cell Wall Acetylation on Corn Stover Hydrolysis by
Cellulolytic and Xylanolytic Enzymes. Cellulose 2009, 16, 711.
(14) Chen, X.; Shekiro, J.; Elander, R.; Tucker, M. Improved Xylan
Hydrolysis of Corn Stover by Deacetylation with High Solids Dilute
Acid Pretreatment. Ind. Eng. Chem. Res. 2012, 51, 70.
(15) Mitchell, D.; Grohmann, K.; Himmel, M.; Dale, B.; Schroeder,
H. Effect of the Degree of Acetylation on the Enzymatic Digestion of
Acetylated Xylans. J. Wood Chem. Technol. 1990, 10, 111.
Authors
Jie Wu − Forest Products Biotechnology/Bioenergy Group,
Department of Wood Science, Faculty of Forestry, University of
British Columbia, Vancouver, BC V6T 1Z4, Canada
Kwang Ho Kim − Clean Energy Research Center, Korea
Institute of Science and Technology, Seoul 136-791, Republic of
Korea; orcid.org/0000-0003-3943-1927
Chang Soo Kim − Clean Energy Research Center, Korea
Institute of Science and Technology, Seoul 136-791, Republic of
Korea
Yunqiao Pu − Center for Bioenergy Innovation, Joint Institute of
Biological Science, Biosciences Division, Oak Ridge National
Laboratory, Oak Ridge, Tennessee 37830, United States;
orcid.org/0000-0003-2554-1447
Arthur J. Ragauskas − Center for Bioenergy Innovation, Joint
Institute of Biological Science, Biosciences Division, Oak Ridge
National Laboratory, Oak Ridge, Tennessee 37830, United
States; Department of Chemical and Biomolecular Engineering
& Department of Forestry, Wildlife and Fisheries, Center for
Renewable Carbon, University of Tennessee, Knoxville,
Tennessee 37996, United States; orcid.org/0000-00023536-554X
Complete contact information is available at:
https://pubs.acs.org/10.1021/acssuschemeng.9b07226
Notes
The authors declare no competing financial interest.
ACKNOWLEDGMENTS
The authors are grateful for the financial support from the
Natural Science and Engineering Council of Canada (NSERC)
and the Korea Institute of Science and Technology (KIST).
The authors would also like to thank Novozymes (Davis, CA)
for the generous donation of enzymes. Mr. Junjie Wang and
Miss Hui Zhu are thanked for their contributions during their
stay at the Forest Products Biotechnology/Bioenergy group as
research interns. This manuscript has been authored, in part
(AJR and YP), by UT-Battelle, LLC under Contract No. DEAC05-00OR22725 with the U.S. Department of Energy. The
United States Government retains and the publisher, by
accepting the article for publication, acknowledges that the
United States Government retains a nonexclusive, paid-up,
irrevocable, worldwide license to publish or reproduce the
published form of this manuscript, or allow others to do so, for
United States Government purposes. The Department of
Energy will provide public access to these results of federally
sponsored research in accordance with the DOE Public Access
Plan (http://energy.gov/downloads/doe-public-access-plan).
The views and opinions of the authors expressed herein do
■
5853
https://dx.doi.org/10.1021/acssuschemeng.9b07226
ACS Sustainable Chem. Eng. 2020, 8, 5847−5855
ACS Sustainable Chemistry & Engineering
pubs.acs.org/journal/ascecg
Research Article
(37) dos Santos, A. C.; Ximenes, E.; Kim, Y.; Ladisch, M. R. Lignin−
Enzyme Interactions in the Hydrolysis of Lignocellulosic Biomass.
Trends Biotechnol. 2019, 37, 518.
(38) Li, X.; Li, M.; Pu, Y.; Ragauskas, A. J.; Klett, A. S.; Thies, M.;
Zheng, Y. Inhibitory Effects of Lignin on Enzymatic Hydrolysis: The
Role of Lignin Chemistry and Molecular Weight. Renewable Energy
2018, 123, 664.
(39) Pan, X.; Xie, D.; Gilkes, N.; Gregg, D. J.; Saddler, J. N.
Strategies to Enhance the Enzymatic Hydrolysis of Pretreated
Softwood with High Residual Lignin Content. Appl. Biochem.
Biotechnol. 2005, 124, 1069.
(40) Tu, M.; Chandra, R. P.; Saddler, J. N. Evaluating the
Distribution of Cellulases and the Recycling of Free Cellulases during
the Hydrolysis of Lignocellulosic Substrates. Biotechnol. Prog. 2007, 23
(2), 398−406.
(41) Chen, X.; Shekiro, J.; Franden, M. A.; Wang, W.; Zhang, M.;
Kuhn, E.; Johnson, D. K.; Tucker, M. P. The Impacts of Deacetylation
Prior to Dilute Acid Pretreatment on the Bioethanol Process.
Biotechnol. Biofuels 2012, 5, 8.
(42) Chen, X.; Wang, W.; Ciesielski, P.; Trass, O.; Park, S.; Tao, L.;
Tucker, M. P. Improving Sugar Yields and Reducing Enzyme
Loadings in the Deacetylation and Mechanical Refining (DMR)
Process through Multistage Disk and Szego Refining and Corresponding Techno-Economic Analysis. ACS Sustainable Chem. Eng.
2016, 4 (1), 324−333.
(43) Tunc, M. S.; Van Heiningen, A. R. P. Hydrothermal
Dissolution of Mixed Southern Hardwoods. Holzforschung 2008,
DOI: 10.1515/HF.2008.100.
(44) Li, H.; Saeed, A.; Jahan, M. S.; Ni, Y.; Van Heiningen, A.
Hemicellulose Removal from Hardwood Chips in the Pre-Hydrolysis
Step of the Kraft-Based Dissolving Pulp Production Process. J. Wood
Chem. Technol. 2010, 30 (1), 48−60.
(45) Hu, J.; Arantes, V.; Saddler, J. N. The Enhancement of
Enzymatic Hydrolysis of Lignocellulosic Substrates by the Addition of
Accessory Enzymes Such as Xylanase: Is It an Additive or Synergistic
Effect? Biotechnol. Biofuels 2011, 4, 36.
(46) Zhai, R.; Hu, J.; Saddler, J. N. The Inhibition of Hemicellulosic
Sugars on Cellulose Hydrolysis Are Highly Dependant on the
Cellulase Productive Binding, Processivity, and Substrate Surface
Charges. Bioresour. Technol. 2018, 258, 79.
(47) Ju, X.; Engelhard, M.; Zhang, X. An Advanced Understanding
of the Specific Effects of Xylan and Surface Lignin Contents on
Enzymatic Hydrolysis of Lignocellulosic Biomass. Bioresour. Technol.
2013, 132, 137−145.
(48) Johansson, L. S.; Campbell, J. M.; Koljonen, K.; Stenius, P.
Evaluation of Surface Lignin on Cellulose Fibers with XPS. Appl. Surf.
Sci. 1999, 144-145, 92.
(49) Tshabalala, M. A. Chapter 8: Surface Characterization. Handb.
wood Chem. wood Compos 2005, 217.
(50) Bendzalova, M.; Pekarovicova, A.; Kokta, B. V.; Chen, R.
Accessibility of Swollen Cellulosic Fibers. Cellul. Chem. Technol. 1996,
30 (1−2), 19−32.
(51) Ogiwara, Y.; Arai, K. Swelling Degree of Cellulose Materials
and Hydrolysis Rate with Cellulase. Text. Res. J. 1968, 38 (9), 885−
891.
(52) Stone, J. E.; Scallan, A. M.; Donefer, E.; Ahlgren, E.
Digestibility as a Simple Function of a Molecule of Similar Size to
a Cellulase Enzyme. Adv. Chem. Ser. 1969, 95, 219−241.
(53) Grethlein, H. E. The Effect of Pore Size Distribution on the
Rate of Enzymatic Hydrolysis of Cellulosic Substrates. Bio/Technology
1985, 3, 155.
(54) Yu, X.; Atalla, R. H. A Staining Technique for Evaluating the
Pore Structure Variations of Microcrystalline Cellulose Powders.
Powder Technol. 1998, 98 (2), 135−138.
(55) Kumar, R.; Mago, G.; Balan, V.; Wyman, C. E. Physical and
Chemical Characterizations of Corn Stover and Poplar Solids
Resulting from Leading Pretreatment Technologies. Bioresour.
Technol. 2009, 100, 3948.
(16) Kong, F.; Engler, C. R.; Soltes, E. J. Effects of Cell-Wall Acetate,
Xylan Backbone, and Lignin on Enzymatic Hydrolysis of Aspen
Wood. Appl. Biochem. Biotechnol. 1992, 34−35 (1), 23−35.
(17) de Groot, B.; van Dam, J. E. G.; van ’t Riet, K. Alkaline Pulping
of Hemp Woody Core: Kinetic Modelling of Lignin, Xylan and
Cellulose Extraction and Degradation. Holzforschung 2009, 49 (4),
332−342.
(18) Karp, E. M.; Donohoe, B. S.; O’Brien, M. H.; Ciesielski, P. N.;
Mittal, A.; Biddy, M. J.; Beckham, G. T. Alkaline Pretreatment of
Corn Stover: Bench-Scale Fractionation and Stream Characterization.
ACS Sustainable Chem. Eng. 2014, 2 (6), 1481−1491.
(19) Chen, X.; Shekiro, J.; Elander, R.; Tucker, M. Improved Xylan
Hydrolysis of Corn Stover by Deacetylation with High Solids Dilute
Acid Pretreatment. Ind. Eng. Chem. Res. 2012, 51 (1), 70−76.
(20) Min, D. Y.; Jameel, H.; Chang, H. M.; Lucia, L.; Wang, Z. G.;
Jin, Y. C. RSC Adv. 2014, 4, 10845−10850.
(21) Grabber, J. H.; Hatfield, R. D.; Lu, F.; Ralph, J. Coniferyl
Ferulate Incorporation into Lignin Enhances the Alkaline Delignification and Enzymatic Degradation of Cell Walls. Biomacromolecules
2008, 9 (9), 2510−2516.
(22) Nakagame, S.; Chandra, R. P.; Kadla, J. F.; Saddler, J. N. The
Isolation, Characterization and Effect of Lignin Isolated from Steam
Pretreated Douglas-Fir on the Enzymatic Hydrolysis of Cellulose.
Bioresour. Technol. 2011, 102 (6), 4507−4517.
(23) Rahikainen, J. L.; Martin-Sampedro, R.; Heikkinen, H.; Rovio,
S.; Marjamaa, K.; Tamminen, T.; Rojas, O. J.; Kruus, K. Inhibitory
Effect of Lignin during Cellulose Bioconversion: The Effect of Lignin
Chemistry on Non-Productive Enzyme Adsorption. Bioresour.
Technol. 2013, 133, 270−278.
(24) Jiang, W.; Xu, J. A Novel Stepwise Pretreatment on Corn Stalk
by Alkali Deacetylation and Liquid Hot Water for Enhancing
Enzymatic Hydrolysis and Energy Utilization Efficiency. Bioresour.
Technol. 2016, 209, 115.
(25) Mok, Y. K.; Arantes, V.; Saddler, J. N. A NaBH Coupled
Ninhydrin-Based Assay for the Quantification of Protein/Enzymes
During the Enzymatic Hydrolysis of Pretreated Lignocellulosic
Biomass. Appl. Biochem. Biotechnol. 2015, 176 (6), 1564−1580.
(26) Katz, R. P.; Scallan, A. M. The Determination of Strong and
Weak Acidic Groups in Sulfite Pulps. Sven. papperstidning 1984, 87,
48−53.
(27) Chandra, R. P.; Saddler, J. N. Use of the Simons’ Staining
Technique to Assess Cellulose Accessibility in Pretreated Substrates.
Ind. Biotechnol. 2012, 8 (4), 230−237.
(28) Laine, J.; Stenius, P.; Carlsson, G.; Ström, G. Surface
Characterization of Unbleached Kraft Pulps by Means of ESCA.
Cellulose 1994, 1, 145.
(29) Yao, L.; Yoo, C. G.; Meng, X.; Li, M.; Pu, Y.; Ragauskas, A. J.;
Yang, H. A Structured Understanding of Cellobiohydrolase i Binding
to Poplar Lignin Fractions after Dilute Acid Pretreatment. Biotechnol.
Biofuels 2018, DOI: 10.1186/s13068-018-1087-y.
(30) Liu, E.; Li, M.; Das, L.; Pu, Y.; Frazier, T.; Zhao, B.; Crocker,
M.; Ragauskas, A. J.; Shi, J. Understanding Lignin Fractionation and
Characterization from Engineered Switchgrass Treated by an Aqueous
Ionic Liquid. ACS Sustainable Chem. Eng. 2018, 6, 6612.
(31) Garrote, G.; Domínguez, H.; Parajó, J. C. Study on the
Deacetylation of Hemicelluloses during the Hydrothermal Processing
of Eucalyptus Wood. Holz als Roh - und Werkst. 2001, 59, 53.
(32) Zanuttini, M.; Marzocchi, V. Kinetics of Alkaline Deacetylation
of Poplar Wood. Holzforschung 1997, 51 (3), 251−256.
(33) Giummarella, N.; Pu, Y.; Ragauskas, A. J.; Lawoko, M. A
Critical Review on the Analysis of Lignin Carbohydrate Bonds. Green
Chem. 2019, 21, 1573.
(34) Sun, R. C.; Tomkinson, J. Comparative Study of Lignins
Isolated by Alkali and Ultrasound-Assisted Alkali Extractions from
Wheat Straw. Ultrason. Sonochem. 2002, 9 (2), 85−93.
(35) Fengel, D.; Wegener, G. Wood: Chemistry, Ultrastructure,
Reactions. Holz als Roh-und Werkstoff 1984, 42, 314.
(36) Biermann, C. J. Handbook of Pulping and Papermaking 1996,
101.
5854
https://dx.doi.org/10.1021/acssuschemeng.9b07226
ACS Sustainable Chem. Eng. 2020, 8, 5847−5855
ACS Sustainable Chemistry & Engineering
pubs.acs.org/journal/ascecg
(56) Chundawat, S. P. S.; Donohoe, B. S.; Da Costa Sousa, L.; Elder,
T.; Agarwal, U. P.; Lu, F.; Ralph, J.; Himmel, M. E.; Balan, V.; Dale, B.
E. Multi-Scale Visualization and Characterization of Lignocellulosic
Plant Cell Wall Deconstruction during Thermochemical Pretreatment. Energy Environ. Sci. 2011, 4 (3), 973−984.
(57) Gupta, V. K.; Schmoll, M.; Herrera-Estrella, A.; Upadhyay, R.
S.; Druzhinina, I.; Tuohy, M. G. Biotechnology and Biology of
Trichoderma 2014, 325.
(58) Mao, J. D.; Holtman, K. M.; Franqui-Villanueva, D. Chemical
Structures of Corn Stover and Its Residue after Dilute Acid
Prehydrolysis and Enzymatic Hydrolysis: Insight into Factors
Limiting Enzymatic Hydrolysis. J. Agric. Food Chem. 2010, 58, 11680.
(59) Mueller-Harvey, I.; Hartley, R. D.; Harris, P. J.; Curzon, E. H.
Linkage of P-Coumaroyl and Feruloyl Groups to Cell-Wall
Polysaccharides of Barley Straw. Carbohydr. Res. 1986, 148 (1),
71−85.
(60) Smith, M. M.; Hartley, R. D. Occurrence and Nature of Ferulic
Acid Substitution of Cell-Wall Polysaccharides in Graminaceous
Plants. Carbohydr. Res. 1983, 118 (C), 65−80.
(61) Sjöström, E.; Janson, T.; Haglund, P.; Enström, B. The Acidic
Groups in Wood and Pulp as Measured by Ion Exchange. In Journal of
Polymer Science Part C: Polymer Symposia; Wiley Online Library:
1965; Vol. 11, pp 221−241.
(62) Lindströ m, T.; Carlsson, G. The Effect of Chemical
Environment on Fiber Swelling. Sven. Papperstindning-Nordisk Cellul.
1982, 85 (3), 14−20.
(63) Gierer, J. Chemical Aspects of Kraft Pulping. Wood Sci. Technol.
1980, 14, 241.
(64) Chakar, F. S.; Ragauskas, A. J. Ind. Crops Prod. 2004, 20, 131−
141.
(65) Jensen, A.; Cabrera, Y.; Hsieh, C.; Nielsen, J.; Ralph, J.; Felby,
C. Holzforschung 2017, 71 (6), 461−469.
(66) Das, P.; Sto, R. B.; Area, M. C.; Ragauskas, A. J. Effects of OneStep Alkaline and Two-Step Alkaline/Dilute Acid and Alkaline/Steam
Explosion Pretreatments on the Structure of Isolated Pine Lignin.
Biomass Bioenergy 2018, 120 (November 2018), 350−358.
(67) Guerra, A.; Filpponen, I.; Lucia, L. A.; Saquing, C.;
Baumberger, S.; Argyropoulos, D. S. Toward a Better Understanding
of the Lignin Isolation Process from Wood. J. Agric. Food Chem. 2006,
54 (16), 5939−5947.
(68) Li, M.; Foster, C.; Kelkar, S.; Pu, Y.; Holmes, D.; Ragauskas, A.;
Saffron, C. M.; Hodge, D. B. Structural Characterization of Alkaline
Hydrogen Peroxide Pretreated Grasses Exhibiting Diverse Lignin
Phenotypes. Biotechnol. Biofuels 2012, 5, 1−15.
(69) Song, Y.; Chandra, R.; Zhang, X.; Tan, T.; Saddler, J.
Comparing Deep Eutectic Solvent (DES) to Hydrotropes for Their
Ability to Enhance the Fractionation and Enzymatic Hydrolysis of
Willow and Corn Stover. Sustain. Energy Fuels 2019, 3, 1329.
(70) Takada, M.; Niu, R.; Minami, E.; Saka, S. Characterization of
Three Tissue Fractions in Corn (Zea Mays) Cob. Biomass Bioenergy
2018, 115 (April), 130−135.
(71) Ma, R.; Guo, M.; Zhang, X. Selective Conversion of Biorefinery
Lignin into Dicarboxylic Acids. ChemSusChem 2014, 7, 412.
(72) Xiang, Q.; Lee, Y. Y. Oxidative Cracking of Precipitated
Hardwood Lignin by Hydrogen Peroxide. Appl. Biochem. Biotechnol.
2000, 84-86, 153.
(73) Dupont, A. L.; Egasse, C.; Morin, A.; Vasseur, F.
Comprehensive Characterisation of Cellulose- and LignocelluloseDegradation Products in Aged Papers: Capillary Zone Electrophoresis
of Low-Molar Mass Organic Acids, Carbohydrates, and Aromatic
Lignin Derivatives. Carbohydr. Polym. 2007, 68, 1.
(74) Abdelaziz, O. Y.; Brink, D. P.; Prothmann, J.; Ravi, K.; Sun, M.;
García-Hidalgo, J.; Sandahl, M.; Hulteberg, C. P.; Turner, C.; Lidén,
G.; et al. Biological Valorization of Low Molecular Weight Lignin.
Biotechnol. Adv. 2016, 34, 1318.
(75) del Rio, L. F.; Chandra, R. P.; Saddler, J. N. The Effects of
Increasing Swelling and Anionic Charges on the Enzymatic
Hydrolysis of Organosolv-Pretreated Softwoods at Low Enzyme
Loadings. Biotechnol. Bioeng. 2011, 108 (7), 1549−1558.
Research Article
(76) Zhong, N.; Chandra, R.; Saddler, J. J. N. Sulfite Post-Treatment
To Simultaneously Detoxify and Improve the Enzymatic Hydrolysis
and Fermentation of a Steam-Pretreated Softwood Lodgepole Pine
Whole Slurry. ACS Sustainable Chem. Eng. 2019, 7, 5192−5199.
5855
https://dx.doi.org/10.1021/acssuschemeng.9b07226
ACS Sustainable Chem. Eng. 2020, 8, 5847−5855