José
Adelson Santana Neto1, Juliana Silva de Oliveira2, Edson
Mauro Santos2, Elizabete Cristina Batista da Costa2, Carla
Aparecida Soares Saraiva2, Ricardo Martins
Araújo Pinho3, Alexandre Fernandes Perazzo3* and Celso
José Bruno de Oliveira2,4
1Universidade
Federal de Sergipe, Av. Marechal Rondon, s/n, Jd. Rosa Elze. São Cristóvão -
SE, Brazil
2Universidade
Federal da Paraíba, Centro de Ciências Agrárias, Campus II, Rodovia BR 079, Km
12, Areia - PB, Brazil
3Universidade
Federal do Maranhão, BR-222, KM 04, S/N, Boa Vista, Chapadinha, MA – Brazil
4Global One Health initiative (GOHi), Ohio State University (OSU),
Columbus, Ohio, USA
*For
correspondence: alexandreperazzo@hotmail.com
Received
17 June 2020; Accepted 26 September 2020; Published 10 January 2021
Abstract
The aim of this study was to evaluate the effects of different sources
of nitrogenous compounds on the in vitro utilisation
of neutral detergent fibre from buffel grass in advanced phenological stage, the
experiment consisted of testing five levels of substitution of urea for casein:
0, 25, 50, 75 and 100%. The effects of the substitution levels were evaluated
by in vitro incubation at different
times: 0, 3, 6, 9, 12, 24, 36, 48, 72 and 96 h. The degradation rate of
potentially degradable NDF increased up to the replacement level of 50%, but
declined by 6.53 and 13.57% in the treatments with 75 and 100% substitution of
urea for casein, respectively, as compared with the treatment without
substitution. Discrete lag time was reduced by 1.31 h in the treatment with 50%
substitution and by 2.7 h at 100% substitution, as compared with 0%
substitution. The substitution of up to 50% non-protein nitrogen for true
protein increased microbial growth efficiency by 16.1% as compared with the
treatment without substitution. Acetate and propionate concentrations were not
affected by the substitution of urea for casein. The use of 50% non-protein
nitrogen and 50% true protein as nitrogen sources for rumen microorganisms
favour microbial growth and optimise the degradation of neutral detergent fibre
from low-protein buffel grass. © 2021 Friends Science Publishers
Keywords: Ammonia; Casein; Rumen; Urea
Introduction
Tropical grasses produce large amounts of dry matter all year long.
However, at certain times of the year, such as in the drought period, the fibre
and protein contents of those forages typically increase and decrease,
respectively, resulting in lower digestibility and nutritional quality (Arruda
et al. 2010).
Buffel grass (Cenchrus
ciliares) is a species adapted to the soil-climatic conditions of arid
regions of the world, where it has the potential to be used in livestock
systems by virtue of its great drought resistance. Notwithstanding this fact,
the rapid phenological development of this species in the drought period leads
to a reduction in its protein value, with crude protein (CP) contents reaching
around 3% (Santos et al. 2005). On the other hand, neutral detergent
fibre (NDF) contents increase under those circumstances, easily surpassing 70%
on a dry matter basis.
The use of non-protein nitrogen (NPN) at levels
exceeding 27% of the total CP of the diet has shown to support satisfactory
production performance in ruminants (Mallmann et al. 2006). For cellular multiplication to occur, the
microbial flora requires peptides, amino acids, and ammonia, which are
hydrolysed from a source of true protein or NPN (Kanjanapruthipong and Leng
1998). Therefore, studies addressing the effects of different sources of
nitrogenous compounds on microbial growth and putative changes in the digestion
of the fibrous carbohydrates could provide valuable information to improve the
utilisation of the fibrous fractions of buffel grass during the drought period
of the year.
In this study, we investigated the effects of
different sources of nitrogenous compounds on the in vitro utilisation of neutral detergent fibre.
Materials
and Methods
The experiment was carried out at the Laboratory of Forage Crops of the
Department of Animal Science, Centre for Agrarian Sciences, Federal University
of Paraíba (UFPB), located in Areia - PB, Brazil. A rumen-fistulated goat was
used as a donor of rumen fluid. The goat was fed elephant grass only for seven
consecutive days prior to rumen-fluid collection in order to reduce the
concentration of nitrogenous compounds in the rumen fluid.
The experimental procedures were previously approved
by the Ethics Committee on the Use of Animals (CEUA) of the Centre for
Biotechnology (CBiotec) at UFPB (approval no. 0209/14), which are in accordance with the resolutions of the National Council
for Control of Animal Experimentation (CONSEA).
Buffel grass (Cenchrus Ciliares)
in advanced phenological stage was collected from a deferred pasture. The grass
was dried in a forced-air oven (60ºC) and ground in a knife mill with 2-mm
sieves for the incubation procedures and in a knife mill with 1-mm sieves for
dry matter determinations (DM; method 930.15), crude protein (CP; method
968.06), ether extract (EE; 954.05), and mineral matter (MM; method 942.05) as
proposed by AOAC (2012). Neutral detergent fibre (NDF), acid detergent fibre
(ADF), and lignin contents were determined (Soest 1967) and corrected for ash
and nitrogenous compounds. Neutral detergent insoluble nitrogen was expressed
as a proportion of total nitrogen (NDIN/TN), as previously described (Licitra et al. 1996). Total carbohydrates (TC) were estimated by the following equation:
TC (%) = 100 – (%CP + %EE + %MM). Non-fibrous carbohydrates (NFC) were
calculated as NFC = 100 – (%CP + %NDFap + %MM + %EE), where NDFap is NDF free
of ash and protein, as described by Sniffen et al. (1992) (Table 1).
The inoculum containing active microbial populations
was obtained from rumen fluid sampled three hs after first feeding. The fluid
was saturated with carbon dioxide (CO2) and incubated at 39ºC. The
intermediate phase was collected, centrifuged at 500 rpm for 10 min, and
supernatant was discarded in order to obtain the inoculum containing active
microbial population (Russell and Martin 1984). The pellet was resuspended
another two times in autoclaved McDougall buffer (9.80 g NaHCO3;
4.65 g Na2HPO4*2H2O; 0.57 g KCl; 0.12 g MgSO4*7H2O;
and 0.04 g CaCl2, diluted with distilled water up to the volume of
1000 mL).
The experiment consisted of testing five levels of
substitution of non-protein nitrogen (NPN) (urea) for true protein (casein).
Urea (9.58 mg) was added so that ammonia nitrogen concentration in the rumen
fluid was 17.76 mg dL–1, corresponding to the treatment with 100%
NPN. The urea was used as a source of NPN, and casein AR (Dinâmica Química
Contemporânea Ltd., Brazil) was used as a source of true protein. After the
ammonia nitrogen concentration was defined, the experimental levels were
obtained through fractional replacements of urea (NPN) by casein.
The experiment was set up as a completely randomised
design with five treatments and three replicates. The treatments contained the
following proportions of nitrogen sources: 100% urea-derived nitrogen (9.59 mg)
and 0% casein (0 mg); 75% urea (7.20 mg) and 25% casein (2.39 mg); 50% urea
(4.80 mg) and 50% casein (4.80 mg); 25% urea (2.39 mg) and 75% casein (7.20
mg); and 0% urea (0 mg) and 100% casein (9.59 mg). In addition to the nitrogen
source, each replicate (incubation bottle) consisted of growth medium (28 mL of
McDougall buffer and 7 mL of inoculum) and 350 mg buffel grass. Bottles
containing growth medium only (35 mL) served as blank. In vitro digestibility and microbial growth parameters were
determined in triplicate per treatment at each sampling time. The 35 mL of the nitrogen
sources were used.
Three bottles without inoculum served as blank for
digestibility determinations.
Each bottle was then saturated with CO2,
capped, and sealed. Bottles were incubated in a BOD (Biochemical Oxygen Demand)
incubator for 96 h at 39ºC. Samplings were performed at 0, 3, 6, 9, 12, 24, 48,
72 and 96 h of incubation. Produced gases were removed from all bottles in
these 3-h intervals using syringes. At the
end of each incubation time, the bottles were removed from the BOD incubator
and the residue was filtered for NDF degradability determinations. A 2.0-mL
sample of growth medium was collected from each experimental unit, placed in
microtubes and centrifuged at 5200 rpm for 10 min. Supernatant was then frozen for
later analysis of the concentration of ammonia nitrogen (N-NH3). The pellet was
resuspended in NaCl solution (0.9% w/v) and centrifuged at 5200 rpm for 10 min;
the supernatant was discarded; and the pellet was resuspended again in NaCl
solution (0.9% w/v) and frozen for later determination of microbial protein.
Ammonia concentration was determined by a colorimetric method (Chaney and
Marbach 1962), whereas microbial protein content was obtained following the
method of Bradford (1976).
For volatile
fatty acids (VFA) analysis, a 2.0-mL sample of growth medium was collected from
all experimental units at 48 h of incubation, transferred to microtubes, and
centrifuged at 5200 rpm for 10 min. The supernatant was then frozen for VFA
profiling by means of high-performance liquid chromatograph (HPLC) (SHIMADZU,
SPD-10A VP) coupled to an ultraviolet (UV) detector operating at a wavelength
of 210 nm. A C18 column (SHIMADZU) with 30 cm × 7.9 mm diameter and 0.6 mL min–1 flow was used under a pressure of 69 kgf, with
the water mobile phase in 1% orthophosphoric acid and injected volume of 20 µL. Acetate, propionate, and butyrate
concentrations; acetate/propionate ratio; total VFA and lactate concentrations
were determined.
Blanks
(bottles containing the incubation solutions without substrate) were also
incubated to adjust the existing variations. The bottles were closed using
rubber corks and their contents were homogenized by agitation. In order to determine the NDF degradability at each
sampling period, the residual material from each bottle was
collected and washed with warm water in a filtering crucible until growth
medium was removed. This residue was dried in an air oven and, weighed on an
analytical scale after 24 h. The NDF content, considering the indigestible part of the feed, was determined
from this residue by the method of Soest (1967).
The NDF residues at the different times, for each
treatment, were analysed by the Gauss-Newton algorithm and adjusted to the
non-linear logistic model described by Milgen et al. (1991) and Detmann
et al. (2011).
(I)
Where, Rt = undegraded NDF residue at time “t” (%); U = potentially
degradable fraction of NDF (pdNDF) (%); I = undegradable fraction of NDF (iNDF)
(%); c = fractional rate of degradation of pdNDF (h–1); p =
fractional rate of lag time (h–1); and t = time (h).
The function described in (I) is considered
symmetrical in relation to the fractional degradation rates c and p, the lowest
values of which are frequently known to be associated with c (Vieira et al.
1997). However, when the fractional rates c and p tend towards the same
estimate, mathematical indeterminacy will be observed, and the model should be
re-parameterised according to L’Hôspital’s rule (Milgen et al. 1991):
(II)
Where, λ = combined fractional rate of lag time and degradation (h–1).
In this situation, because parameter λ simultaneously describes the
lag-time and degradation rates, the fractional rate of degradation was
determined from λ, using the gamma-2 distribution properties (Ellis et al. 1994):
c’= 0.59635 x λ (III)
Where, c’ = fractional rate of degradation of pdNDF (h–1) for
the cases in which the re-parameterised model is used (Equation II).
Discrete lag time was obtained following the models of
Vieira et al. (1997):
(IV)
Where, L = discrete lag time (h); R(0) = undegraded NDF residue at t = 0
(%); R(ti) = undegraded NDF residue obtained at the inflection point of the degradation
(%); μ = derivative of the degradation curve adjusted to the inflection
point (maximum rate of degradation of the substrate) (h–1); ti =
time corresponding to the inflection point of the degradation curve (h).
The ti values were calculated according to the
observations of Milgen et al. (1991) (Equations I and II, respectively):
(V)
(VI)
The specific microbial growth
rate in relation to pdNDF was calculated in accordance with the hypothesis
proposed by Beuvink and Kogut (1993):
(VII)
Where, Sgr = specific microbial
growth rate (h–1). After the Sgr estimates were calculated, the
microbial growth efficiencies in relation to pdNDF were estimated by following
the theories of Pirt (1965):
(VIII)
Where, Y = microbial efficiency
(g cells g degraded carbohydrates–1); m = requirement for the
maintenance of microorganisms (g carbohydrates g cells–1 h–1);
and Ym = theoretical maximum efficiency of the microorganisms on the substrate (g cells g
degraded carbohydrates–1). The Ym parameter was adopted as
reference, with the value of 0.4 g cells g–1 degraded
carbohydrates, while m was set as 0.05 g carbohydrates g cells–1 h–1,
as recommended by Russell et al. (1992).
The
effectively degraded fractions of NDF were calculated as proposed by Costa
et al. (2008), in an adjusted version of the methodology described by
Ørskov and McDonald (1979):
(IX)
Where, EDF: effectively degraded
fraction of NDF (%); ƒ(t) = function relative to the displacement flow of solids in
the rumen environment. To define the function described in (IX), we assumed
ruminal displacement flow of solids with gamma-1 distribution (Ellis et al. 1994), to which the hypothetical values of 0.020, 0.035, and 0.050 were
allocated.
In this way,
in the context of the equations (X), EDF was calculated as follows:
(X)
The models were fitted to the
degradation profiles as a function of the different substitution levels and
were compared descriptively. The N-NH3 and microbial protein concentrations
obtained at the incubation times of 0 and 48 h were evaluated by variance and
regression analyses. The criteria used in the choice of the model were the
significance of regression coefficients at 5% probability by Tukey’s test and
the determination coefficient (r2), which was obtained as the sum of regression
squares divided by the sum of squares of treatments and biological phenomenon.
Volatile fatty
acid and lactate data were subjected to variance and regression analyses. The
criteria for the choice of the regression models were the significance of the
regression parameters, determination-coefficient values, and the biological
interpretation of the regression curves. The variables were analysed
statistically by Tukey’s test at the 5% significance level.
The asymptotic standard deviation
(ASD) was calculated from the root mean residual square of each model. Table 1:
Chemical composition of buffel grass, urea, and casein
Item |
Forage |
Urea |
Casein |
Dry matter (g kg–1) |
854.4 |
982.1 |
900.0 |
Organic matter (g kg DM–1) |
905.2 |
997.6 |
972.4 |
Ash (g kg DM–1) |
94.8 |
2.4 |
27.6 |
Crude protein (g kg DM–1) |
49.8 |
2610.0 |
889.7 |
Ether extract (g kg DM–1) |
16.6 |
- |
3.2 |
Total carbohydrates (g kg DM–1) |
838.8 |
- |
- |
1NDF (g kg DM–1) |
857.0 |
- |
- |
2NDFap (g kg DM–1) |
799.7 |
- |
- |
3ADF (g kg DM–1) |
348.1 |
- |
- |
4NFC (g kg DM–1) |
39.1 |
- |
- |
5TN (g kg DM–1) |
8.0 |
- |
- |
6NDIN (g kg DM–1) |
195.6 |
- |
- |
Lignin (g kg DM–1) |
76.6 |
- |
- |
1Neutral detergent fibre; 2NDF free of ash or protein; 3Acid
detergent fibre; 4Non-fibrous carbohydrates; 5Total
nitrogen; 6Neutral detergent insoluble nitrogen
Table 2: Substitution of non-protein
nitrogen (NPN) for true protein (TP) on the concentrations of ammonia nitrogen
and microbial protein at 0 and 48 h of in
vitro incubation
Parameter |
Substitution
of NPN for TP (%) |
CV (%)1 |
R2 |
P-value |
|||||
|
0 |
25 |
50 |
75 |
100 |
|
|
L |
Q |
N-NH3
(mg dL–1) |
|||||||||
0 h2 |
7.58 |
7.15 |
6.17 |
5.63 |
1.69 |
13.55 |
0.80 |
0.01 |
Ns |
48 h3 |
26.0 |
24.80 |
22.64 |
19.91 |
19.25 |
17.34 |
0.97 |
0.02 |
Ns |
Microbial
protein (mg L–1) |
|||||||||
0 h4 |
161.33 |
162.00 |
162.05 |
163.03 |
161.33 |
31.51 |
- |
ns |
Ns |
48 h5 |
463.33 |
536.01 |
622.66 |
494.65 |
442.54 |
10.76 |
0.79 |
ns |
0.02 |
1CV = coefficient of variation, significant at the 5% probability level (P < .05 by Tukey’s test); NS = not
significant; L = linear; Q = quadratic, R² = determination coefficient. 2Ŷ=8.3+0.053X;
3Ŷ= 26.20–0.073X; 4Ŷ=161.9; 5Ŷ=
462.11+4.97X–0.053X2
Table 3: Substitution of non-protein
nitrogen (NPN) for true protein (TP) on the pH of the medium at 0 and 48 h of in vitro incubation
Parameter |
Substitution
of NPN for TP |
CV(%)1 |
R2 |
P-value |
|||||
|
0 |
25 |
50 |
75 |
100 |
|
|
L |
Q |
pH |
|||||||||
0 h |
7.10 |
7.14 |
7.17 |
7.16 |
7.19 |
1.94 |
- |
ns |
ns |
48 h |
7.29 |
7.26 |
7.28 |
7.22 |
7.25 |
0.47 |
- |
ns |
ns |
1 Coefficient of variation
All statistical
analyses, both linear and non-linear, were performed using SAS software
(Statistical Analysis System).
Results
The mean rumen ammonia values
varied between 1.69 and 7.58 mg dL–1 at 0h and between 19.91 and 26.0 mg dL–1 at 48 h (Table 2). All treatments provided sufficient uptake of ammonia
for the cellulose- and hemicellulose-degrading microorganisms. After 48 h of
incubation, ammonia values decreased linearly (P < .05) from 26.0 to 19.25 mg dL–1 as per the
substitution for true protein increased from 0 to 100% (Fig. 1a).
At the beginning of incubation (0 h), microbial
protein did not differ across the treatments (P > .05) averaging 161.9 mg L–1. However, at 48 h of
incubation, the treatments fitted a quadratic model (P < .05), with maximum microbial protein attained at 46.88% of
substitution of NPN for true protein, according to the derivation of the
second-degree equation (Table 2, Fig. 1b).
No significant effects of substitution or incubation
time were observed (P > .05) on
the pH of the medium (Table 3), which averaged 7.15 and 7.26 at 0 and 48 h of
incubation, respectively.
Rumen concentrations of acetate, propionate, and
lactate and acetate/propionate ratio did not differ (P > .05) according to the levels of replacement of urea by
casein (Table 4). The respective variables averaged 51.5, 21.4, 0.45, and 2.46
mM.
Butyrate levels increased linearly (P < .05), from 0.87 to 2.05 mM, as
urea was replaced with casein (0 and 100% substitution, respectively).
The highest concentration of total VFA (80.57 mM) was observed at 50% replacement of
NPN. Supplementation with 50% TP increased the degradation of the fibrous
fraction (pdNDF) (Table 5), which consequently led to higher concentrations of
total VFA.
The replacement of non-protein nitrogen (urea) with a
source of true protein (casein) increased the degradation rate of pdNDF up to
the substitution level of 50%. The treatment with 50% substitution showed a higher fractional rate of degradation
resulting from the transformation of parameter λ, revealing a 17.42%
increase compared with the treatment with 0% substitution. The degradation rate
of pdNDF was declined by 6.53 and 13.57% in the treatments in which 75 and 100%, respectively of the NPN were
replaced with TP (Table 5).
The treatment in which 50% of the NPN was substituted
for TP provided a 1.31 h shorter estimate of discrete lag time than the
treatment with 0% substitution and a 2.7 h shorter value compared with full
substitution. Lag time declined by 1.31 h until the substitution level of 50%.
Supplementation with the different nitrogenous
compounds increased the specific growth rate of microorganisms only by 4.5% up
to the substitution level of 50% (Table 6). However, this variable then
decreased 10.9 to 24.9% from 75 to 100% substitution. The treatment in which
50% of NPN was replaced with TP provided the best results for microbial growth,
which was 17.4% more efficient than in the treatment with 0% substitution. When,
100% of NPN was replaced with TP, the specific growth rate of microorganisms
decreased by 13.7%.
The efficiency of microbial growth on pdNDF (g
microbial DM kg degraded carbohydrate–1) behaved similarly to the
other evaluated parameters. The substitution of up to 50% provided an
approximately 16.1% more efficient microbial growth (363.37 g microbial DM kg
degraded carbohydrate–1). Full substitution of NPN for TP, in turn,
led to a 3.3% reduction in this variable in comparison with the treatment
without substitution.
The highest estimates for effective degradation of
pdNDF were observed in the treatment with 0% substitution, in which the
effectively degraded fraction of pdNDF would increase by 20.7% at the passage
rate of 0.035 h–1 as compared with the treatment with 100% substitution.
This increased would reach up to 22.6% using a passage rate of 0.05 h–1
(Table 7).
At the end of the incubation trial, NDF degradation
responded quadratically, reaching its highest value at around 42.03% of
substitution of NPN for true protein, based on the derivation of the equation (Fig.
2).
Discussion
The mean rumen ammonia values at
48 h of incubation (Table 2) in all treatments were higher
than the minimum threshold of 4 to 5 mg dL–1 recommended by Satter
and Slyter (1974) for degradation of NDF. The present values are also above the
10 mg dL–1 recommended by Soest (1994) for adequate microbial growth
on carbohydrates and for optimum NDF degradation.
In the treatment with 100% substitution, the N-NH3
concentration of 10 mg dL–1 was attained at 24 h of incubation,
whereas the other treatments, containing different proportions of casein and
urea, reached this minimum concentration at 9 h of incubation (Fig. 1a). This
had an impact on microbial growth, which was lower throughout the incubation
period when nitrogen originated only from the true protein (Fig. 1b). A
possible explanation for this finding is the fact that urea is more efficient
in providing larger levels of ammonia nitrogen than casein when equal levels of
protein are supplemented (Zorzi et al. 2009).
According to Leng (1990), 10 to 20 mg N-NH3
dL–1 are necessary for maximising rumen degradation of low-quality
tropical grasses. This N-NH3 concentration improves the efficiency
of microbial synthesis by 15 to 28%, regardless of the nitrogen source
(Kanjanapruthipong and Leng 1998). In the present study, the longest time to
reach the minimum N-NH3 value necessary for maximum NDF degradation
was observed for the treatment with 100% substitution of NPN.
Table 4: Concentrations of volatile
fatty acids (VFA) and lactate according to the substitution of non-protein
nitrogen (NPN) for true protein (TP)
VFA2 |
Substitution of NPN for TP |
||||
0% |
25% |
50% |
75% |
100% |
|
Acetate |
51.6 |
51.8 |
53.5 |
50.4 |
50.2 |
Propionate |
20.8 |
21.30 |
24.9 |
20.0 |
20.0 |
Butyrate |
0.87 |
0.94 |
1.56 |
1.61 |
2.05 |
Lactate |
0.39 |
0.49 |
0.47 |
0.41 |
0.47 |
A/P3 |
2.48 |
2.43 |
2.16 |
2.62 |
2.60 |
Total VFA |
73.27 |
74.04 |
79.96 |
72.01 |
72.20 |
Parameter |
Regression equation |
CV (%) |
L |
Q |
R2 |
Acetate |
Ŷ = 51.5 |
8.4 |
0.317 |
0.326 |
- |
Propionate |
Ŷ = 21.4 |
14.8 |
0.491 |
0.152 |
- |
Butyrate |
Ŷ = 0.81+ 0.01X |
24.2 |
0.001 |
0.88 |
0.90 |
Lactate |
Ŷ = 0.45 |
23.6 |
0.707 |
0.500 |
- |
A/P3 |
Ŷ = 2.46 |
20.6 |
0.634 |
0.488 |
- |
Total VFA |
Ŷ=73.3+0.2X–0.002X2 |
1.1 |
0.001 |
0.001 |
0.58 |
1Levels of substitution of urea for casein; 2Concentration of
VFA in millimolar (mM); 3Acetate/Propionate
ratio
Table 5: Estimates of rumen degradation
parameters of potentially degradable neutral detergent fibre and asymptotic
standard deviations (ASD) for the degradation profiles adjusted according to
the substitution of non-protein nitrogen for true protein
Parameter1 |
Substitution level |
||||
0% |
25% |
50% |
75% |
100% |
|
U (%) |
43.6 |
40.99 |
38.8 |
41.5 |
37.8 |
λ (h–1) |
0.1955 |
0.2134 |
0.2295 |
0.1826 |
0.1689 |
c’ (h–1)2 |
0.1165 |
0.1272 |
0.1368 |
0.1089 |
0.1007 |
RVDR (%)3 |
100 |
109.18 |
117.42 |
93.47 |
86.43 |
L (h) |
8.79 |
8.05 |
7.48 |
9.41 |
10.18 |
ASD |
9.60 |
9.01 |
8.61 |
9.25 |
9.87 |
U = potentially degradable fraction of NDF (pdNDF);
λ = common fractional rate of lag time and degradation; c’ = fractional
rate of degradation obtained from the conversion of parameter λ; RVDR =
relative value of the degradation rate; L = discrete lag time. 2Estimated
according to gamma-2 distribution properties: c’ = 0.59635λ. 3Relative
value of the degradation rate in relation to the forage (0 mg dL–1).
Table 6: Secondary parameters associated
with microbial growth on the potentially degradable neutral detergent fibre
according to the substitution of non-protein nitrogen for true protein.
Parameter |
Substitution level |
||||
0% |
25% |
50% |
75% |
100% |
|
μ1 |
3.13 |
3.22 |
3.27 |
2.79 |
2.35 |
Sgr |
0.0719 |
0.0785 |
0.0844 |
0.0671 |
0.0621 |
EMG |
312.95 |
348.78 |
363.37 |
308.15 |
302.55 |
1μ = maximum
degradation rate (h–1); Sgr = specific microorganism growth rate (h–1);
EMG = efficiency of microbial growth on pdNDF (g microbial DM kg degraded
carbohydrate–1)
Diets formulated with different nitrogen sources that
meet the rumen-degradable protein requirements can improve the uptake of
nutrients to the most diverse groups of rumen microorganisms, increasing the
efficiency of microbial protein synthesis. Furthermore, as shown in Fig. 1,
these diets allow a more synchronous release of nitrogen sources for microbial
growth. Bowen et al. (2016) found no differences regarding the source
used (urea or casein) on the efficiency of microbial protein synthesis using a
low-quality tropical grass. In this same study, there was a difference in the
amount of casein used to maximise the efficiency of microbial synthesis, which
was only increased when a greater uptake of digestible organic matter was
provided. This improvement was associated with a four-fold increase in the
concentration of N-NH3, in the rumen fluid, resulting from greater
degradation of the dietary protein. The presence of true protein is important
in the synthesis of amino acids by cellulolytic bacteria such as branched-chain
volatile fatty acids (Bowen et al. 2016); however, they also use ammonia
as a nitrogen source to synthesise microbial protein, which is likely explained
by the greater microbial protein synthesis seen in the 50% substitution
treatment.
All pH values found remained above the minimum limits
for fibrolytic activity (Ørskov 1986). For Martins et al.
(2006), pH values higher than 6.0 favour the maintenance of an adequate rumen
medium for cellulolytic bacteria to adhere to the particles (Cysneiros et
al. 2013). Rasmussen et al. (1989) did not observe effects of pH
changes between 6.0 and 8.0 on bacterial adherence, indicating that pH values
slightly above 7.0 may favour NDF degradability.
According to Júnior et al. (2004), decreased
ammonia production is expected to increase propionate production and a
consequent decrease in the acetate/propionate ratio in the rumen. However, no
such effect was observed in the present study. Despite the different N-NH3
concentrations at the different urea and casein ratios, there was no change in
pH values, which is a key factor to the proliferation of cellulolytic
microorganisms (Russell and Wilsom 1996), the main producers of acetate. As a
result, the fermentation of the substrate used becomes uniform regardless of
the NPN and TP ratios.
Table 7: Estimates of effectively
degraded fraction of potentially degradable neutral detergent fibre (% of
pdNDF) according to the substitution of non-protein nitrogen for true protein
Treatment |
Rumen passage rate (h–1)1 |
||
|
0.020 |
0.035 |
0.050 |
0% |
35.88 |
31.36 |
27.65 |
25% |
34.27 |
30.26 |
26.91 |
50% |
32.85 |
29.22 |
26.17 |
75% |
33.73 |
29.24 |
25.59 |
100% |
30.28 |
25.99 |
22.55 |
1 Assuming ruminal displacement flow kinetics of solids with gamma-1
distribution.
Fig. 1: Effect of substitution of non-protein nitrogen (NPN)
for true protein (TP) on the concentrations of ammonia (a) and microbial protein (b)
over 96 h of in vitro incubation
Fig. 2: Degradation of NDF (%)
according to the substitution of the nitrogenous-compound source
The molar proportions of acetate and propionate were
68.8% and 28.2%, respectively, which are within the normal ranges of 54 to 74%
(acetate) and 16 to 27% (propionate) proposed by Silva and Leão (1979) and by
Filho and Pina (2011). Although the present study was conducted in a closed and
restricted system (in vitro) and
despite the fact that the rumen is a dynamic environment, with passage of
solids and liquids and entry of saliva and feed, our results corroborate in vivo studies (Heldt et al.
1999; Laguna et al. 2013; Gonçalves et al. 2015).
Butyrate concentrations increased because the bacteria
that use the butyrate pathway for the reoxidation of NADH2 usually
have only this pathway for VFA production, having no enzymes that are able to
utilise other mechanisms to generate another end product (Moss et al. 2000). In this way,
butyrate-producing cellulolytic bacteria show affinity in the use of the
products from the fermentation of amino acids and small peptides derived from
the degradation of true protein; e.g. branched-chain VFA.
Our results regarding total VFA concentrations and
individual quantities of each VFA contrast with those reported by Xin et al. (2010), who did not observe
differences in the concentrations of total VFA produced from diets with
different protein sources (soy protein isolate, livestock urea, and
encapsulated urea). However, these treatments significantly changed the molar
percentages of individual VFA, with the urea-based diets resulting in larger
acetate and smaller propionate proportions in comparison with the soybean
meal-based diet, leading to an increase in the acetate/propionate ratio.
The N-NH3 levels and the supply of a
true-protein source have a direct influence on the fermentation of the
substrates present in the rumen, since these compounds participate in the
synthesis of nitrogenous bases and serve as donors of carbon backbones,
respectively. This explains the increase in total VFA when these compounds were
combined at the substitution level of 50%.
The highest concentration of total VFA was observed in
the treatment with 50% substitution. This can be explained by the fact that the
supply of a true-protein source, such as casein, is important for fermentation
and microbial growth, since amino acids provide carbon backbones when degraded.
Within addition to ammonia, which is generated by the hydrolysis of urea,
carbon backbones are used for the synthesis of microbial protein (Ribeiro et al. 2014). Detmann et al.
(2011) demonstrated 24% and 96% increases in fibre degradation with the supply
of 1/3 and 1/2 TP in comparison with treatments with urea addition and without
addition of any nitrogenous compounds, respectively.
The discrete lag time observed in our study can be
attributed to some factors. One of them is the ammonia concentration in the
rumen fluid. According to Detmann et al. (2009), inefficiency in the
concentration of ammonia in the rumen fluid may lead to a microbial deficiency
in the synthesis of compounds necessary for microbial adherence on the fibre or
production of enzymes to initiate the fibre degradation. Other important
factors that possibly explain the higher degradation rate of pdNDF and lower
discrete lag time in combined-supplementation situations are the constant
maintenance of high ammonia values in the medium, favouring cellulose- and
hemicellulose-degrading bacteria, and providing the requirements of the many
species of the rumen environment. In general, fibrous carbohydrate-fermenting
cellulolytic and hemicellulolytic bacteria use ammonia nitrogen as the main source
of nitrogen for microbial growth. However, non-fibrous carbohydrate-fermenting
bacteria use amino acids as a nitrogen source. Because the incubation medium in
the present study was rich in fibrous carbohydrates (Table 1), the treatments
providing larger amounts of TP compromised effective fibre degradation.
According to Kozloski (2011), amino acids are
catabolised and converted to branched-chain fatty acids (isobutyrate,
isovalerate) by bacteria with high deaminating activity. These are essential
substrates for the growth of fibrous carbohydrate-degrading bacteria,
increasing the potential of pdNDF fermentation and generating a higher
concentration of VFA, which are responsible for 70–80% of the energy available
to the ruminant.
Franco et al. (2004) stated that increasing
concentrations of ammonia nitrogen favour the proliferation of fibrous
carbohydrate-degrading bacteria, increasing the pdNDF degradation rate. Ammonia
is of critical importance for the degradation of carbohydrates, since it is
used by microorganisms that degrade the cellulose and hemicellulose from the
plant cell wall for cellular growth and multiplication Russell et al.
(1992). However, besides ammonia, those microorganisms also need branched-chain
fatty acids (isovalerate, isobutyrate) that originate from the degradation of
branched-chain proteins, such as leucine, isoleucine, and valine, for the
synthesis of microbial proteins (Haraguchi et al. 2006). Therefore, it can be affirmed that the
interaction between urea and casein provided the best conditions for NDF
degradation, since the treatment containing equal amounts of the two
nitrogenous compounds had the best degradation rates.
Sampaio et al. (2009) mentioned that the
requirement of nitrogenous compounds by rumen microorganisms is approximately
7% CP, and that values lower than this compromise microbial growth. The basal
CP content of 4.98% found in the forage used in the present experiment is lower
than the recommended above-mentioned value.
Similar results were found by Zorzi et al.
(2009), who observed a deleterious effect of casein inclusion, where a 0.5 mg
mL–1 increment resulted in a 1.1% higher rate of pdNDF degradation.
However, the use of casein at levels higher than 1.0 and 2.0 mg mL–1
had an inhibitory effect on the estimates of this parameter compared with the
treatment containing forage only, reducing this variable by 6.4 and 9.1%. The
same authors found that supplementation with urea only, irrespective of the
level, increased the degradation rate of pdNDF.
According to Detmann et al. (2011), the maximum
values found for potentially degradable NDF and microbial efficiency were
achieved when the non-protein nitrogen and true protein ratios were 2/3 and
1/3. According to these authors, protein supplement balancing optimises the
degradation of NDF from low-quality forages for cattle. Another parameter that
can be associated with improved utilisation of NDF in relation to the use of
NPN and TP is discrete lag time (L). Detmann et al. (2011) described
discrete lag time as the estimate (by approximation) of the time required for
the events preceding the NDF degradation activities, which involve hydration,
fixation to the substrate, and enzyme synthesis.
Higher efficiency in microbial protein production has
considerable importance in ruminant nutrition. Fernandes et al. (2015)
mentioned that microbial protein is considered to be of high biological value,
with 62.5% crude protein, 60% of which is true and available and contains the
complete amino acid profile for ruminants, in addition to accounting for 50 to
80% of the protein absorbable in the intestine (Bach
et al. 2005). Given these facts, the
data demonstrate the importance of adequate supplementation with NPN and
true-protein sources for rumen microorganisms, since they are critically
important for animal’s biological response. In addition to helping degrade the
feed, the lager number of microorganisms present which serve as a source of
proteins to the host animal.
Because it is a parameter derived directly from the
degradation rate of pdNDF, the effectively degraded fraction of pdNDF should
respond similarly to the other studied parameters. However, no such trend was
observed in the present study. Although the potentially degradable fraction of
NDF (U) is dependent of the substrate (forage) (Detmann et al. 2011),
different values are assigned to each treatment according to the type and
utilisation of nitrogenous supplementation, aiming to increase the potentially
degradable fraction and consequently reduce the undegradable fraction. This
occurs because supplementation with different types of nitrogenous compounds
modifies the rumen medium, which may or may not promote an environment that
allows for better degradation of NDF. A difference is thus observed in the
effectively degraded fraction of pdNDF regarding degradation rates:
supplementation with non-protein nitrogen and true protein benefits the
digestion of the fibre from buffel grass both in the extent of its degradation
by the rumen microorganisms and in the synthesis of microbial protein (Costa
et al. 2008).
Conclusion
The use of 50% non-protein nitrogen and 50% true protein as the nitrogen
source for rumen microorganisms optimises the degradation of neutral detergent
fibre from low-quality buffel grass and microbial growth in vitro. Further in vivo
studies are warranted to test this hypothesis.
Author Contributions
JSO and CJBO
designed the project. JASN and JSO wrote the manuscript. JSO, CJBO, CASS, EMS
and ECBC designed the methodology and collected the data. CASS, RMAP and EMS
conceptualized the idea for this work and critically revised the manuscript.
CJBO, JSO and AFP approved the final version of the manuscript.
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