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ORIGINAL PAPER
Optimization of Phytosterols Recovery from Soybean OilDeodorizer Distillate
Feng Yan • Haojun Yang • Jianxin Li • Huiling Wang
Received: 4 October 2011 / Revised: 19 January 2012 / Accepted: 19 January 2012 / Published online: 8 February 2012
� AOCS 2012
Abstract A large amount of phytosterols in the bound
form remains in the waste residue during the traditional
process of recovering tocopherols and sterols from soybean
oil deodorizer distillate (SODD). In order to avoid the loss
of natural resources, we developed a process to recover the
maximum amount of phytosterols from SODD. The pro-
cess includes saponification, methyl esterification, and
crystallization. The purpose of saponification and methyl
esterification were to decompose the bound phytosterols
and to esterify the fatty acids, respectively. The yield of
sterols was dependent on saponification and solvent crys-
tallization. The conditions of saponification and solvent
crystallization were optimized by single-factor tests and
response surface methodology, respectively. The sterol
yield obtained under the optimized conditions was 6.64%.
This value is much greater than 4.43% obtained by the
traditional industrial process. The purity of the recovered
sterols was 94.7%.
Keywords Soybean oil deodorizer distillate (SODD) �Phytosterols � Steryl esters � Crystallization � Response
surface methodology
Introduction
Phytosterols (plant sterols) structurally resemble choles-
terol, but with different side-chain configurations. Phytos-
terols are integral natural components of cell membranes in
vegetable oils, nuts, seeds, and grains and are additives in
functional foods (e.g. margarines). Phytosterols have a
wide spectrum of biological effects including anti-inflam-
matory, anti-oxidative, and anti-carcinogenic activities [1].
Their cholesterol-lowering capacities have been exten-
sively researched. Several studies have shown that plant
sterols inhibit intestinal absorption of cholesterol, thereby
lowering total plasma cholesterol [2].
Deodorizer distillates from edible oils constitute a major
industrial source of phytosterols [3]. Deodorization is the last
step in the refining of edible oils and involves the removal of
some undesirable components of natural fats and oils. The
treatment is conducted at 200 �C in vacuo for several hours.
The by-product thus obtained is called ‘‘deodorizer distillate’’
and consists of a complex mixture of various compound
families including fatty acids, sterols, tocopherols, sterol
esters, glycerides, hydrocarbons and others. Soybean oil
deodorizer distillate (SODD) is especially interesting due to
the large amount of useful products it contains, and is an
important source of natural tocopherols and phytosterols [4].
Preparing high-purity concentrates of phytosterols and
tocopherols involves a series of physical and chemical
treatment steps. Several studies have been conducted to
recover phytosterols and tocopherols from deodorization
distillate, such as crystallization [5, 18], solvent extraction
F. Yan (&) � H. Wang
State Key Laboratory of Hollow Fiber Membrane Materials
and Processes, School of Environmental and Chemical
Engineering, Tianjin Polytechnic University,
Tianjin 300160, People’s Republic of China
e-mail: [email protected]
H. Yang
E-Tech Energy Technology Development Corporation,
Tianjin, People’s Republic of China
J. Li (&)
Laboratory for Membrane Materials and Separation Technology,
Sustainable Technology Research Center, Shanghai Advanced
Research Institute, Chinese Academy of Sciences,
Shanghai 201203, People’s Republic of China
e-mail: [email protected]
123
J Am Oil Chem Soc (2012) 89:1363–1370
DOI 10.1007/s11746-012-2023-0
[6], supercritical fluids extraction [7, 8], supercritical
extraction with a multistage countercurrent column [9],
transesterification to form methyl esters followed by frac-
tional distillation [10], neutralization and washing [11],
membrane separation [12], enzymatic esterification [13,
14], and batch adsorption [15]. Phytosterols cannot be
removed by molecular distillation because their molecular
weights and volatilities are similar to those of tocopherols
[16]. It is difficult to recover concentrates of tocopherols
and phytosterols in good yield and high quality. Since
phytosterols are insoluble in some cold solvents, they could
be obtained by crystallization [13].
In industry production, a comprehensive process is
widely adopted. The process includes methyl esterification
by using sulfuric acid as a catalyst, transesterification by
using an alkaline catalyst, crystallization and filtration to
separate sterols, and molecular distillation to produce
concentrated tocopherols, fatty acid methyl esters (FAME)
and waste residue; however, there are two key problems in
the process. One is the low content of tocopherols (about
50%) in the concentrated fractions. The other is that a large
amount of bound sterols (namely sterol esters) is lost in the
waste residue [17]. The percentages of sterols (in the bound
form) are about 30, 17, and 20% of waste residue from
CGOG TECH. Bioengineering Co. Ltd. (Tianjin, China);
Heilongjiang Jiusan Oil & Fat Co. Ltd. (Heilongjiang
Province, China,); and Jiangsu Spring Fruit Biological
Products Co. Ltd. (Jiangsu Province, China), respectively.
The purpose of the present study was to develop a suitable
process to recover phytosterols not only in free state, but
also in the bound form from SODD.
Materials and Methods
Materials
Soybean oil deodorizer distillate and a standard sample of
mixed phytosterols (95.30% phytosterols) were supplied by
CGOG TECH. Bioengineering Co. Ltd. (Tianjin, China).
Cholesterols ([97% purity) were purchased from Tianjin
Guangfu Fine Chemical Research Institute (Tianjin,
China). Other chemicals, such as acetic anhydride, pyri-
dine, methanol, ethanol, n-propanol, petroleum ether, ace-
tone, butanone, cyclohexanone, benzene, toluene, were all
of analytical grade and were used as received.
Reaction Procedure
Saponification of SODD
Soybean oil deodorizer distillate (30 g) was dissolved in
30 mL ethanol in a 250-mL three-neck flask equipped
with a reflux condenser, a dropping funnel, and a nitrogen
duct. After the mixture was heated to reflux, NaOH
solution (30 mL) was added dropwise through the drop-
ping funnel. The mixture reacted at reflux temperature and
under N2 for 2 h after adding NaOH. After saponification,
excess acid was added to the mixture. The acidified
mixture was then transferred to a separatory funnel, and
the organic phase was washed with water three times. The
residue water in the organic phase was evaporated under
vacuum. The fatty acid steryl esters in SODD were
transformed into free sterols and FFA, and the glycerides
were transformed into FFA and glycerol. In order to
decompose the steryl esters completely, the effects of
NaOH dosage on the free sterol content in the organic
phase after saponification and acidify was investigated by
using single-factor tests. Two replicates for each dosage
of NaOH were done to obtain mean sterol contents in the
organic phases.
Methyl Esterification
The organic phase obtained after saponification was
esterified with methanol catalyzed by using sulfuric acid.
After esterification, the mixture was repeatedly washed
with water until pH 7 was achieved. During the process, the
FFA were then transformed into FAME. The organic phase
was then evaporated under vacuum.
Phytosterol Recovery by Crystallization
Phytosterols were recovered from the feed solution
obtained after saponification and methyl esterification by
using solvent crystallization. The feedstock was dissolved
in different solvents at 60 �C. Then the solution was
cooled to a ripening temperature and was kept at this
temperature for a ripening time. Phytosterol crystals were
finally obtained by vacuum filtration. The solvent selec-
tion, ripening temperature, and ripening time were varied
to optimize the crystallization conditions by using a
central-composite design (CCD). The independent factors
A, B and C represented proportion of feed solution to
solvent, ripening temperature (�C), and ripening time (h),
respectively. Five levels (-1.68, -1, 0, ?1 and ?1.68)
CCD was performed to determine the best combination
effect of the three crystallization parameters. The layout
of the CCD and the experimental response (sterols yield,
%) obtained with each run are shown in Table 1 and all
experiments were randomized. Two replicates were done
for each run to obtain the mean yield of sterols. The
fitting degree of the model was evaluated by the coef-
ficient of determination (R2) and the analysis of variance
(ANOVA).
1364 J Am Oil Chem Soc (2012) 89:1363–1370
123
Analytical Methods
Determination of Sterol Yield
The yield of sterols was calculated by using Eq. 1.
Sterol yield
¼ the mass of phytosterols recovered from SODD=
the mass of SODD ð1Þ
Determination of Sterol Content
A GC (Agilent 6890N, USA) with an HP-5 capillary col-
umn was used to analyze the content of sterols in the feed
solution and in the sterol products. All samples were
derivatized with acetic anhydride before testing. Choles-
terol was used as an internal standard. Analytical condi-
tions were: 280 �C column temperature; 300 �C FID
detector; N2 carrier gas; and temperature program of 1 min
at 100 �C, followed by heating to 250 �C at 35 �C/min, and
then to 280 �C at 30 �C/min (where it was held for
30 min).
The purity of sterols was calculated by using Eq. 2 [17]
Y ¼ FAsample � minternal
Ainternal � msample
� 100% ð2Þ
where Y is the content of sterols (%), F is the correction
factor, Asample is the total peak area of sterols in a sample,
Ainternal is the total peak area of internal standard, minternal is
the mass of the internal standard (mg), and msample is the
mass of a sample (mg). The correction factor F was
obtained from the standard sample (95.30% purity) from
CGOG TECH. Bioengineering Co., Ltd.
Results and Discussion
The free sterol content in SODD was 4.36% and increased
to 9.30% in the feed solution after SODD was saponified
and to 9.12% in the feed solution after methyl esterifica-
tion. More than one-half of the sterols was in the bound
form in SODD. Furthermore, the free sterol content was
6.80% in the feed solution after methyl esterification and
transesterification in industrial production from CGOG
TECH. Bioengineering Co. Ltd. The yield of sterols was
only 4.43% in the industrial production. The results indi-
cate that the present process including saponification can
transfer the bound sterols into free sterols more efficiently,
and the process is promising for sterol recovery from
SODD.
Optimization of Saponification
The dosage of NaOH for the saponification was explored
as shown in Fig. 1. NaOH dosage influenced the
Table 1 The setting of central
composite design and the
observed response values
Run Code parameter Actual parameter values Yield of sterols
Y (%)A B C A (g/ml) B (�C) C (h)
1 -1.00 -1.00 -1.00 2.00 0.00 16.00 5.64
2 0.00 0.00 0.00 3.00 5.00 24.00 6.58
3 0.00 0.00 0.00 3.00 5.00 24.00 6.60
4 0.00 -1.68 0.00 3.00 -3.41 24.00 6.04
5 0.00 0.00 1.68 3.00 5.00 37.45 6.26
6 -1.00 -1.00 1.00 2.00 0.00 32.00 5.64
7 -1.00 1.00 1.00 2.00 10.00 32.00 5.75
8 0.00 0.00 -1.68 3.00 5.00 10.55 6.72
9 0.00 0.00 0.00 3.00 5.00 24.00 6.58
10 1.00 -1.00 -1.00 4.00 0.00 16.00 6.16
11 1.00 1.00 1.00 4.00 10.00 32.00 6.24
12 0.00 0.00 0.00 3.00 5.00 24.00 6.64
13 0.00 0.00 0.00 3.00 5.00 24.00 6.68
14 1.00 -1.00 1.00 4.00 0.00 32.00 6.46
15 -1.68 0.00 0.00 1.32 5.00 24.00 5.72
16 0.00 1.68 0.00 3.00 13.41 24.00 5.84
17 1.68 0.00 0.00 4.68 5.00 24.00 6.37
18 1.00 1.00 -1.00 4.00 10.00 16.00 5.52
19 -1.00 1.00 -1.00 2.00 10.00 16.00 5.44
20 0.00 0.00 0.00 3.00 5.00 24.00 6.68
J Am Oil Chem Soc (2012) 89:1363–1370 1365
123
decomposition of bound sterols. The free sterol content in
the feed solution after saponification, C (%), increased
from 6.64 to 9.30% as the NaOH/SODD mass ratio
increased from 0.17/1 to 0.33/1. The free sterol content did
not increase further with an increased NaOH/SODD ratio.
Therefore, the optimized dosage of NaOH for the saponi-
fication was 0.33/1 NaOH/SODD mass ratio.
In order to confirm whether there was unreacted sterol
ester left in the organic phase, column chromatography was
used to separate free sterols from the organic phase when
the NaOH/SODD mass ratio was 0.33:1. The FTIR spec-
trum of decomposed SODD after separating free sterols is
presented in Fig. 2, where the C=O and C–O–C stretching
bands of the ester group were 1,744 and 1,168 cm-1,
respectively (curve A) and the two wave peaks disappeared
when SODD was saponified (curve B). This result indi-
cated that there was no/little unreacted sterol esters left in
the organic phase after saponification.
Phytosterol Recovery by Crystallization After Methyl
Esterification
Selection of Solvents for Crystallization
In the present work, a variety of solvents including various
alcohols, alkanes, ketones, esters, and aromatics were used
in the crystallization of phytosterols from feed solution
after methyl esterification (Table 2). Methanol gave the
best crystallization efficiency with high yield (4.48%) and
high purity (95.33%). When alcohols or ketones were used
as crystallization solvents, the yield of phytosterols
decreased as the length of hydrocarbon chains increased.
No phytosterols crystals precipitated in n-propanol and
butanone, probably due to increased solubility of sterols as
the hydrocarbon chain length of alcohols and ketones
increased. Furthermore, the sterols crystallized only at low
temperature (-8 �C) when benzene or toluene was used as
solvent. Methanol, petroleum ether and ethyl acetate gave
higher yields of sterols.
As discussed above, low productivity of sterols was
obtained when a single solvent was used for the crystalli-
zation. The yield of phytosterols in a solvent–water system
was much higher than that in a single solvent (Fig. 3). The
yield of phytosterols increased from 3.35 to 6.55% as the
water/petroleum ether ratio (V/V) increased from 0 to 0.16.
This may be because sterols tend to form hydrates with
water, which leads to their decreased solubility. Accord-
ingly, the yield of phytosterols extracted from a water-
bearing feed solution would be much higher than from an
anhydrous feed [18]. As shown, further increases in the
water content in petroleum ether had little effect on phy-
tosterol yield. By contract, the phytosterol yield increased
5
6
7
8
9
10
NaOH/SODD mass ratio (w/w)
C (
%)
0.17:1 0.20:1 0.25:1 0.33:1 0.50:1
Fig. 1 Effect of NaOH dosage on the content of free sterols in feed
solution after saponification
4000 3500 3000 2500 2000 1500 1000 500
2675
2853
2924
723
939
1096
1168
1242
1461
1744
1710
Wavenumber cm-1
Tra
nsm
ittan
ce
A
B
Fig. 2 The FT-IR spectra of SODD oil (A) and decomposed SODD
oil (B)
Table 2 The effects of different solvents on crystallization of
phytosterols
Run Solvents TRa (�C) Yield of sterols (%) Purityb (%)
1 Methanol 6 4.48 95.33
2 Ethanol 6 1.17 93.74
3 n-Propanol 6 No crystal
4 Acetone 6 2.57 91.82
5 Butanone 6 No crystal
6 Benzene -8 2.18 82.86
7 Toluene -8 1.36 91.85
8 Petroleum ether 6 3.35 93.12
9 Ethyl acetate 6 3.20 93.68
a Ripening temperatureb Purity of sterol sample
1366 J Am Oil Chem Soc (2012) 89:1363–1370
123
from 4.48 to 5.68% as water/methanol ratio increased from
0 to 0.12. In the same way, the yield of phytosterols
increased to 5.43% as the water/ethyl acetate ratio was
increased to 0.16. The purities of sterol samples obtained
from the solvent–water systems were all [94%. A petro-
leum ether–water co-solvent system could give higher yield
of sterols. The optimal yield of phytosterols was 6.64% with
95.88% purity at 0.24 water/petroleum ether ratio (V/V).
Optimization of Crystallization Conditions
by Single-Factor Tests
The yield of recovered sterols increased from 4.40% to a
maximum of 6.70% as the feed solution to solvent ratio
increased from 1:2 to 1:0.33 (w/V) (Fig. 4a). The yield of
recovered sterols increased as solvent dosage decreased.
Some sterols remain dissolved in the solvent and do not
precipitate. However, it showed a negative influence on
sterols precipitation with further decrease of solvent dos-
age. As shown in Fig. 4a, at a range from 1:0.33 to 1:0.2,
the yield of recovered sterols decreased as a result of
insufficient phytosterol dissolution. Thus, the optimum
feed solution to solvent ratio was 1:0.33. The sterol yield
decreased as ripening temperature increased, while it
increased when ripening time increased (Fig. 4b, c).
Therefore, the optimum crystallization conditions to obtain
the highest sterol yield were ripening at 5 �C for 24 h.
RSM Model Fitting
RSM was applied to model and optimize the crystallization
conditions of phytosterols recovered from SODD after
saponification and methyl esterification. The significant
quadratic models and the corresponding significant model
term for all responses are tabulated in Table 3.
The best-fitting models were determined through mul-
tiple linear regressions with backward elimination. The
accuracy of the models was evaluated by a coefficient of
determination (R2). The determination coefficient (R2 =
0.8192) indicated that 81.92% of the variation in sterol
yield was attributed to the independent variables (Table 3).
On the other hand, a lower coefficient of variation
(CV = 3.45%) indicated better precision and reliability of
the experiments carried out [19]. The CV as the ratio of the
standard error of estimate to the mean value of the
observed response (as a percentage) was a measure of the
reproducibility of the model and as a general rule a model
is considered to be reasonably reproducible if the CV is not
[10% [20]. By applying diagnostic plots, including normal
probability plotting of residuals, and plotting residuals
versus predicted, assumptions of normality, independence
0.0 0.1 0.2 0.3 0.42
3
4
5
6
7
8
ethyl acetate
petroleum ether
Yie
ld (
%)
Ratio of water/solvent (V/V)
methanol
Fig. 3 Effect of water as a co-solvent on yield of phytosterols by
crystallization
4.0
4.5
5.0
5.5
6.0
6.5
7.0
Proportion of feed solution to solvent (w/V)
Yie
ld (
%)
1:2 1:1 1:0.5 1:0.33 1:0.25 1:0.2
0 5 10 15 204.0
4.5
5.0
5.5
6.0
6.5
7.0
Yie
ld (
%)
Ripening temperature ( oC)
8 16 24 324.0
4.5
5.0
5.5
6.0
6.5
7.0
Yie
ld (
%)
Ripening time (h)
(a)
(b)
(c)
Fig. 4 Effect of crystallization condition single factors on the yield
of phytosterols a ratio of feed solution to solvent, b ripening
temperature, c ripening time
J Am Oil Chem Soc (2012) 89:1363–1370 1367
123
and randomness of the residual were satisfied. The fitted
model for phytosterol yield was accepted. The adequate
precision value was a measure of the ‘‘signal-to-noise
ratio’’ for the responses. A ratio [4 was considered to be
adequate model discrimination [21]. The 6.280 ratio indi-
cated an adequate signal to noise ratio (Table 3). The
predictive model could be used to navigate the space
defined by CCD.
The P value was used as the tool to check the signifi-
cance of each coefficient, which also indicated the inter-
action strength of each parameter. The smaller the P value
was, the greater the significance of the regression coeffi-
cient. In other words, the higher the F value was for the
model, the lower probability that the value was for the
model, which also indicated the greater significance of
the fitted model. In the present study, the model F value of
5.04 indicated the model was significant. There was only a
0.94% chance that a ‘‘Model F-Value’’ this large could
occur due to noise. Values of \0.0500 ‘‘Prob [ F’’ indi-
cated model terms were significant. As shown in Table 3,
the liner term of feed solution to solvent ratio (A) had a
large effect on the sterol yield and was significant due to
the high F value. The quadratic term of feed solution to
solvent ratio, ripening time and ripening temperature were
all significant; however, the effect of interaction between
any two variables did not affect the sterols yield.
Analyzing the contour plots for yield of sterols was the
best way to evaluate the relationships between responses,
variables and interactions. The dimensional response sur-
face was plotted (Fig. 5) as a function of the interaction of
feed solution to solvent ratio (A) and ripening temperature
(B) at a medium ripening time 24 h. With each variable
increasing, the sterol yield initially increased and then
slightly decreased. The responses obtained were convex
Table 3 ANOVA for the
regression model and respective
model terms
Source Sum of
squares
Degree
of freedom
Mean of
square
F value P value
Prob [ FRemarks
Model 2.01 9 0.23 5.04 0.0094 Significant
A 0.49 1 0.49 10.62 0.0082 Significant
B 0.020 1 0.020 0.43 0.5271 Not significant
C 0.20 1 0.20 4.26 0.0660 Not significant
AB 5.000E-003 1 5.000E-003 0.11 0.7492 Not significant
AC 8.450E-003 1 8.450E-003 0.18 0.6782 Not significant
BC 7.200E-003 1 7.200E-003 0.16 0.7016 Not significant
A2 0.72 1 0.72 15.45 0.0028 Significant
B2 0.46 1 0.46 9.93 0.0103 Significant
C2 0.46 1 0.46 9.93 0.0103 Significant
Residual 0.46 10 0.046
Lack of fit 0.45 5 0.091 45.52 0.0004 Significant
Pure error 9.950E-003 5 9.950E-003
R2: 0.8192 CV%: 3.45 Adequate precision: 6.280
10.00
7.50
5.00
2.50
0.002.00 2.50 3.00 3.50 4.00
B: Ripening temperature A
Ratio of feed solution to solvent
Fig. 5 Response surface curve and contour plot showing predicted
response surface of phytosterol yield as a function of feed solution to
solvent ratio and ripening temperature
1368 J Am Oil Chem Soc (2012) 89:1363–1370
123
which suggested well-defined optimum operating condi-
tions. The dimensional response surfaces of interactions
between feed solution to solvent ratio (A) and ripening time
(C), and between ripening temperature (B) and ripening
time (C) were similar to that between feed solution to
solvent ratio (A) and ripening temperature (B).
Optimization of Phytosterol Crystallization Conditions
For crystallization conditions, the RSM clearly indicated
that optimum phytosterol recovery (6.69%) was produced
with a feed solution to solvent ratio (A), ripening temper-
ature (B) and ripening time (C) at 3.41:1 (g/ml), 4.48 �C,
and 26.47 h, respectively. In order to confirm the predicted
results of the optimized model, experiments were carried
out with the crystallization conditions at these conditions.
The sterol yield obtained at the optimized conditions was
6.64%, which suggested the model was reliable. The purity
of recovered phytosterols under the optimized conditions
was 94.7%.
Purity and Structure Analysis of Recovered
Phytosterols
The results from GC analysis of recovered phytosterols
showed that cholesterol (internal standard) and four kinds
of sterols eluted with the relative retention time (RT) of
17.019, 17.875, 19.687, 20.631 and 22.545 min, respec-
tively. According to the peak areas of sterols and Eq. 1, the
purity of the recovered phytosterols sample was 96.95%.
GC–MS spectrometry was further utilized to determine
the exact kind of sterol corresponding to the relative
retention time. Brassicasterols (RT: 17.88 min), campes-
terols (RT: 19.68 min), stigmasterols (RT: 20.63 min) and
b-sitosterols (RT: 22.55 min) were present, which was in
agreement with our previous work [17]. Furthermore, the
brassicasterol, campesterol, stigmasterol, and beta-sitos-
terol contents of the recovered phytosterols were 0.81,
27.72, 23.69 and 44.72 wt%, respectively. In addition, GC–
MS showed that there were impurities in the sterol prod-
ucts; the impurities were sterol derivatives by oxidation/
reduction, such as hydrogenation of sterols.
Conclusions
We developed a saponification, methyl esterification and
solvent crystallization process for phytosterol recovery
from SODD. The conditions of saponification and solvent
crystallization were optimized. Petroleum ether with water
as cosolvent could generate desirable crystallization. The
predicted yield of the recovered sterols (6.69%) was con-
sistent with the experimental result 6.64% (94.7% purity)
under optimum crystallization conditions (3.41:1 g/ml feed
solution to solvent ratio, 26.5 h ripening time, 4.5 �C rip-
ening temperature). Our process is a promising route to
recover phytosterols from SODD.
Acknowledgements The authors gratefully acknowledge the
financial support of the National High Technology Research and
Development Program of China (‘‘863’’ Program, Grant
No.2009AA03Z223), National Science and Technology Major Pro-
ject (2011ZX05011) and Tianjin ‘‘Double Five’’ Science Foundation
(Grant No. SWPY 20080004). The authors also thank Ms. Ming Huo
and Mr. Daogeng Wu for their contributions.
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