Departments of 1Medical Physiology and 2Experimental Medicine, The Panum Institute, University of Copenhagen, DK-2200 Copenhagen, Denmark
Submitted 23 March 2003 ; accepted in final form 16 May 2003
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ABSTRACT |
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dipeptidyl peptidase IV; valine-pyrrolidide; peptide degradation
In recent years, it has been shown that the enzyme dipeptidyl peptidase IV (DPP IV) plays an important role in the in vivo metabolism of two other members of the proglucagon family (GLP-1 and -2) (6, 12, 28) and of the related peptide glucose-dependent insulinotropic polypeptide (GIP) (7, 28). In vitro studies have indicated that high concentrations of glucagon may also be degraded by DPP IV (19, 41), but the significance of this mechanism for glucagon metabolism in vivo has not yet been addressed.
The aim of the present study was, therefore, to examine glucagon metabolism and to identify the sites of its elimination by measurement of arteriovenous concentration differences across organ vascular beds by use of three well-characterized assays specific for different epitopes in glucagon and high-performance liquid chromatography (HPLC). The ability of this approach to reveal metabolic degradation has previously been validated for GLP-1 and GIP (6, 7, 9, 10). In addition, the effect of the selective DPP IV inhibitor valine-pyrrolidide (37) was investigated to ascertain whether DPP IV has a physiological role in glucagon metabolism.
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MATERIALS AND METHODS |
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Because it is known that two other members of the proglucagon family, GLP-1 and -2, are NH2-terminally degraded by DPP IV (6, 12, 28), the susceptibility of glucagon was tested. Glucagon (300 pmol/l) was incubated with recombinant human DPP IV (5 mU/ml, a generous gift from Dr. S. Brenner, Novo Nordisk, Bagsværd, Denmark) in Tris·HCl buffer (600 µl, 0.04 mol/l, pH 7.6) at 37° C for 0, 30, and 120 min (n = 3-4 incubations at each time point). Valine-pyrrolidide [a selective DPP IV inhibitor (34), 0.02 mmol/l, final concentration; a gift from Dr. L. B. Christiensen, Novo Nordisk] was added to additional samples, which were incubated for 30 and 120 min. After incubation, samples were placed in an ice bath, and the reaction was immediately stopped by the addition of trifluoroacetic acid (TFA, 50 µl, 10% vol/vol; Rathburn, Walkerburn, Scotland). Samples were analyzed by reverse-phase HPLC using a C8 column, as previously described for GLP-1 (6) except for the use of a modified gradient of acetonitrile (Rathburn) in 0.1% TFA (0-25% over 5 min, followed by 25-45% over 20 min, and 45-75% over 3 min). Fractions were assayed for glucagon immunoreactivity using antisera 4305 and 4830 as described in Hormonal assays.
Animals and surgical procedures. The animal studies were in accordance with international guidelines (National Institutes of Health publication no. 85-23, revised 1985, and Danish legislation governing animal experimentation, 1987) and were carried out after permission had been granted by the National Superintendence for Experimental Animals.
Danish LYY strain pigs (30-39 kg) were fasted for 24 h before surgery but allowed free access to drinking water. After premedication with ketamine (Ketaminol, 10 mg/kg; Veterinaria, Zurich, Switzerland), the animals were anesthetized with halothane (4% for induction and 1% for maintenance; Halocarbon Laboratories, River Edge, NJ), and maintained with intermittent positive pressure ventilation with an anesthesia ventilator in a semiopen system. Vascular catheters were placed in the right carotid artery for sampling of reference arterial blood and into the pulmonary artery and the left internal jugular, the left femoral, the portal, a hepatic, and the renal veins, as described previously (10). After surgery, animals were heparinized, a saline drip was set up and infused into an ear vein (5 ml/min), and animals were left undisturbed for 30 min.
Glucagon metabolism in vivo. To measure the regional balance of endogenous glucagon (n = 9), arteriovenous concentration differences were measured by taking simultaneous blood samples (4 ml) from the carotid artery and the jugular, renal, and femoral veins. A second set of simultaneous samples was taken from the carotid and pulmonary arteries and the hepatic and portal veins. After a 5-min interval, the protocol was repeated to obtain a duplicate set of samples.
After samples in the basal state had been obtained, glucagon (a gift from Dr. Christian Brand, Novo Nordisk) was dissolved in 0.9% NaCl containing, in addition, 1% human serum albumin (Behringwerke, Marburg, Germany) and infused via the right ear vein catheter at a rate of 5 pmol·kg-1·min-1 for 30 min using a syringe pump. Arterial blood samples were taken at 0, 5, 10, and 15 min after the start of the infusion, after which, during minutes 20-30, two duplicate sets of simultaneous samples were taken from all the vascular sites as described above. After 30 min, the infusion was stopped, and additional arterial blood samples were taken at 1, 2, 4, 6, 10, 15, 20, and 30 min. The total amount of blood taken during the entire procedure was 176 ml, which for a 35-kg pig is 5% of the total blood volume, which has previously been shown not to affect heart rate or blood pressure (10).
In separate experiments (n = 5), the effect of the selective DPP
IV inhibitor valine-pyrrolidide was examined. After premedication with
midazolam (Dormicum, 0.5 mg/kg; Roche, Basel, Switzerland) and ketamine
(Ketaminol, 10 mg/kg; Veterinaria), animals were anesthetized with intravenous
-chloralose (66 mg/kg; Merck, Darmstadt, Germany) and ventilated with
intermittent positive pressure. Animals received two successive glucagon
infusions (1
pmol·kg-1·min-1)
with blood sampling, as above. Sixty minutes after cessation of the first
infusion, valine-pyrrolidide (300 µmol/kg) was given as a bolus intravenous
injection over 2 min. This dose of inhibitor has previously been shown to
inhibit >95% of plasma DPP IV activity for
150 min
(8). Blood samples were taken
at 5-min intervals for 15 min, after which the second glucagon infusion was
started and the protocol repeated for blood sampling.
Blood samples were collected into chilled tubes containing EDTA (7.4 mmol/l, final concentration; Merck) and aprotinin (500 KIU/ml blood; Novo Nordisk), and kept on ice until centrifugation at 4°C. Plasma was separated and stored at -20°C until analysis by radioimmunoassays (RIA), described below.
Hormonal assays. Three different RIAs for glucagon were used. Antiserum 4304 (20, 21) is "side viewing" and directed toward the midregion amino acid sequence 6-15 of glucagon. It binds with equal affinity to all peptides containing this sequence [including PG-(1-69) (glicentin) and PG-(33-69) (oxyntomodulin)], recognizing both COOH- and NH2-terminally truncated or extended forms, and can thus be considered as being largely processing independent. The assay has a detection limit of 2 pmol/l. Antiserum 4305 (20, 21) requires the intact COOH terminus of glucagon and does not cross-react with COOH-terminally truncated or extended molecules (glicentin and oxyntomodulin), making it specific for fully processed glucagon of pancreatic origin. It has a detection limit of 1 pmol/l. Antiserum 4830 was raised in rabbits immunized against the synthetic sequence glucagon-(1-10)-cys, coupled to keyhole limpet hemocyanin with m-maleimidobenzoyl-N-hydroxysuccinimide ester, as described by Dyrberg and Kofod (13). The assay is directed toward the NH2 terminus of glucagon and cross-reacts with oxyntomodulin but <20% with peptides extended from the NH2 terminus of glucagon, including glicentin and PG-(1-61). The assay has an ED50 of 29 ± 4 pmol/l and a detection limit of 2 pmol/l. For all assays, the intra-assay coefficient of variation was <6%. Standard and 125I-labeled glucagon were obtained from Novo Nordisk. Plasma samples were extracted with ethanol (70% vol/vol, final concentration) before assay, giving recoveries of 75%.
Calculations and statistical analysis. For each animal, the net
balance of endogenous glucagon across the brain, hind-limb, kidney, and portal
bed was calculated as a ratio, defined as
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For the liver, the hepatic blood supply was calculated on the assumption
that 75% originates from the portal vein and 25% is of arterial origin. The
net balance across the lungs was defined as
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The extraction of exogenous glucagon was calculated for individual animals as above, after subtraction of the mean endogenous glucagon concentration at each site.
The incremental area under the curve (AUC) for glucagon immunoreactivity
during exogenous infusion was calculated using the trapezoidal method after
substraction of endogenous immunoreactivity in the sample taken before the
start of the infusion. The plasma half-life (t1/2) was
calculated by loge-linear regression analysis of peptide
concentrations in samples collected after termination of the infusion after
subtraction of endogenous arterial glucagon concentrations, and the metabolic
clearance rate (MCR) was calculated using the formula
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The volume of distribution (Vd) was calculated using the formula
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Data are expressed as means ± SE and were analyzed using GraphPAD InStat software, version 1.13 (San Diego, CA) and Statistica software (StatSoft, Tulsa, OK). Two-factor ANOVA for repeated measures with post hoc analysis was used to analyze time course curves. The t1/2, arteriovenous concentration differences, MCR, and Vd were analyzed using ANOVA (where appropriate) and two-tailed t-tests for paired and nonpaired data. One-sample two-tailed tests were used to evaluate organ extractions. P < 0.05 was considered significant.
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RESULTS |
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The susceptibility of glucagon to degradation by DPP IV was examined by incubating the peptide with recombinant human DPP IV. After incubation of glucagon alone, HPLC and analysis of the fractions by NH2-terminal RIA, one minor peak (peak 1) and one major peak (peak 2) were obtained (data not shown). The earlier-eluting peak (peak 1) amounted to 28.9 ± 0.7% of the total immunoreactivity and may represent the oxidized form of glucagon (glucagon contains a methionine residue in the COOH-terminal region that is susceptible to oxidation). Both peaks reduced slowly in size after incubation with recombinant human DPP IV, reaching 88.4 ± 4.4% (peak 1) and 75.7 ± 7.1% (peak 2) of their original size after 120 min, respectively. Peak 1 was not detected with the COOH-terminal assay, but a time-dependent decrease in the size of the peak corresponding to intact glucagon (peak 2, to 76.0 ± 11.6% of its original size after 120 min), together with the appearance of an additional peak (peak 3), was detected. The reductions in size of peaks 1 and 2, together with the formation of peak 3, were totally prevented by coincubation in the presence of valine-pyrrolidide. This suggests that peak 3 is generated specifically as a result of DPP IV-mediated catalysis and may be glucagon-(3-29), which has been reported to be formed after incubation of glucagon with purified porcine renal DPP IV (19, 41). Furthermore, peak 3 was not detectable with the NH2-terminal assay, confirming the specificity of antiserum 4830 and its requirement for the intact NH2 terminus of glucagon.
The catalytic activity of the recombinant enzyme was confirmed by carrying out similar incubations with GLP-1-(7-36) amide instead of glucagon, and HPLC analysis revealed the expected formation of an additional peak eluting in the position of GLP-1-(9-36) amide (data not shown).
Concentrations of glucagon in the basal state. Basal glucagon concentrations differed depending on the assay (ANOVA, P < 0.02). Levels determined with the midregion assay (58 ± 13 pmol/l) did not differ significantly from those determined with the NH2-terminal assay (34 ± 10 pmol/l) but were significantly higher than levels determined with the COOH-terminal assay (16 ± 3 pmol/l, P = 0.01). There was no significant difference in the basal NH2-terminal and COOH-terminal immunoreactivities.
Arteriovenous concentrations of endogenous glucagon. Plasma concentrations of glucagon measured with COOH-terminal (4305), NH2-terminal (4830), and midregion (4304) RIAs are shown in Table 2, and the net balance across the various vascular beds is illustrated in Fig. 1. Renal extraction was detected with all three assays. Extraction across the brain and lung was detected only with the midregion assay. Extraction across the hindlimb was detected only with the COOH-terminal assay. A net secretion of glucagon across the splanchnic bed was detected with both midregion and COOH-terminal assays, and there was a trend (P = 0.066) toward a secretion to be detected with the NH2-terminal assay, whereas the midregion assay detected a modest secretion across the hepatic bed.
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Exogenous glucagon extraction. During infusion of glucagon (5 pmol·kg-1·min-1), arterial glucagon concentrations were similar, irrespective of which assay was used (Fig. 2; incremental plateau concentrations: 365 ± 32, 420 ± 54, and 314 ± 28 pmol/l, ANOVA, P = 0.191; incremental AUC: 11,044 ± 1,040, 11,592 ± 1,386, and 10,967 ± 836 pmol·l-1·min, ANOVA, P = 0.101, midregion and COOH- and NH2-terminal RIAs respectively).
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The plasma concentrations in the different vascular beds achieved during the infusion are shown in Table 3, and the regional extraction is given in Fig. 3. Significant renal extraction was detected with all three assays. Extraction across the hindlimb was detected with the midregion and COOH-terminal assays, with a trend (P = 0.069) for this to be evident with the NH2-terminal assay. Modest hepatic extraction was seen only with the midregion assay. Both the COOH- and NH2-terminal assays detected some extraction across the splanchnic bed, whereas no extraction across the lungs was detectable. Plasma concentrations of glucagon in the jugular vein were greatly elevated during the glucagon infusion due to a "spillover" from the contralateral infusion site in the ear, which precluded calculation of the brain extraction.
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In vivo t1/2 and MCR. Plasma t1/2 values were not significantly different when calculated using COOH-terminal (2.7 ± 0.2 min) or NH2-terminal assays (2.3 ± 0.2 min), but both were shorter (P < 0.02, ANOVA and paired t-test) than the t1/2 calculated using the midregion assay (3.2 ± 0.2 min).
The MCR and distribution volumes were similar irrespective of which assay was used (MCR: 14.4 ± 1.1, 13.6 ± 1.7, and 17.0 ± 1.7 ml·kg-1·min-1; Vd: 68.3 ± 9.0, 51.3 ± 8.3, and 56.1 ± 7.0 ml/kg; midregion, COOH-terminal, and NH2-terminal assays, respectively).
Effect of DPP IV inhibition on glucagon stability in vivo. DPP IV inhibition had no significant effect on the metabolism of either endogenous or exogenous glucagon in vivo (Fig. 4). Thus basal glucagon immunoreactivity (before the start of each infusion) was not significantly altered by DPP IV inhibition (57 ± 7 vs. 50 ± 8, 8 ± 5 vs. 9 ± 6, and 27 ± 6 vs. 29 ± 7 pmol/l; glucagon alone vs. glucagon + valine-pyrrolidide and midregion, COOH-terminal, and NH2-terminal assays, respectively), and arterial glucagon concentrations remained similar during infusion of glucagon alone and together with valine-pyrrolidide (incremental plateau concentration: 44 ± 5 vs. 43 ± 2, 53 ± 7 vs. 43 ± 1, and 32 ± 2 vs. 30 ± 1 pmol/l; incremental AUC: 1,479 ± 240 vs. 1,352 ± 147, 1,434 ± 261 vs. 1,307 ± 83, and 928 ± 17 vs. 908 ± 98 pmol·l-1·min; glucagon alone vs. glucagon + valine-pyrrolidide and midregion, COOH-terminal, and NH2-terminal assays, respectively). The plasma t1/2 and MCR were unaffected by valine-pyrrolidide when determined by midregion (3.2 ± 0.2 vs. 3.1 ± 0.5 min and 15.0 ± 0.9 vs. 16.6 ± 1.1 ml·kg-1·min-1) and COOH-terminal (3.1 ± 0.4 vs. 3.2 ± 0.2 min and 17.1 ± 1.9 vs. 18.4 ± 0.5 ml·kg-1·min-1), but there appeared to be a small trend toward an increase in stability determined with the NH2-terminal assay (2.6 ± 0.3 vs. 2.9 ± 0.5 min and 30.5 ± 4.1 vs. 26.8 ± 1.0 ml·kg-1·min-1), although these changes were not significant.
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DISCUSSION |
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When interpreting the organ extractions of glucagon, it should be borne in mind that the calculations of glucagon extraction are expressed as percent extraction relative to the arterial supply. However, because we did not assess individual organ blood flows, we cannot exclude the possibility that these may have changed during the course of the experiment. Thus, although the percentage of glucagon supplied to each organ that is extracted under endogenous and exogenous conditions can be compared directly, it is possible that the individual organs' contribution to the overall metabolic clearance may vary between the two conditions.
The negative balance (-40%) of glucagon immunoreactivity across the portal bed, detected with all three assays under basal conditions, reflects the net secretion of glucagon from the pancreas and of glicentin and oxyntomodulin from the gut. However, the portal bed also appears to be a site of glucagon removal, since during the infusion an extraction of >10% was detected with the COOH- and NH2-terminal assays. The fact that this was not seen with the midregion assay indicates that the degradation was not extensive, leaving the central sequence of the peptide intact.
The brain and the lung seem not to be major sites of glucagon degradation. Thus, under endogenous conditions, an extraction was detected only with the midregion assay, suggesting either a limited cleavage occurring in the central part of the glucagon molecule or, perhaps, degradation of other endogenous proglucagon products. Given that no extraction of exogenously supplied glucagon was detected in the lung (changes across the brain could not be determined due to a spillover of the infused peptide into the jugular vein from the contralateral infusion site), this would tend to suggest that the pulmonary extraction seen under endogenous conditions may be due to degradation of glicentin, since it was only detected with the midregion assay. The significance of this is unknown.
Degradation across the hindlimb, representing metabolism by connective, supportive, and muscular tissues, was evident, particularly with the COOH-terminal assay (up to 30%) but also with the midregion assay (20%) during exogenous infusion. This would be consistent with the action of neutral endopeptidase (NEP) 24.11, an enzyme with a widespread distribution (17) that has been reported to degrade glucagon in vitro at cleavage sites located predominantly in the midregion and COOH-terminal half of the molecule (24). In support of this, a preliminary study has indicated that a selective inhibitor of NEP 24.11 improves the metabolic stability of glucagon in vivo (45).
A considerable proportion of both endogenous (30%) and exogenous
(>40%) glucagon was removed during passage across the renal bed. During
exogenous glucagon infusion, the renal clearance was calculated after
subtraction of the basal endogenous glucagon immunoreactivity, meaning that
the given values apply to the extraction of the infused glucagon (assuming
that the infusion itself does not affect endogenous glucagon levels). The
corresponding values for endogenous glucagon reflect the renal clearance for
all the glucagon-containing moieties. Glicentin and oxyntomodulin have longer
t1/2 values than glucagon
(27,
32); so it is likely that
their slower metabolic clearance masks the true renal clearance of endogenous
glucagon, thus explaining the difference between the calculated values under
the two conditions (basal and during infusion) in the present study. The fact
that similar renal extractions were revealed by all three assays during the
infusion is indicative of glucagon being substantially degraded to small or
undetectable fragments and not just a limited removal or one or two amino
acids from one or the other terminus. This is in agreement with previously
reported studies of renal metabolism in a number of species, including humans
(14,
22,
30,
40). In the present study,
calculation of the total renal clearance of glucagon (assuming that the
kidneys receive 25% of the cardiac output) gives a value (
320 ml/min)
that is greater than the glomerular filtration rate. Detailed studies have
indicated that this is an active process involving glomerular filtration,
proximal tubular uptake with degradation by tubule brush-border enzymes on the
luminal membrane, and reabsorption of the liberated amino acids, as well as
peritubular uptake (4,
39,
44). The kidney has also been
shown to be an important site of elimination for the related peptides GLP-1
and GIP (7,
10), so renal clearance is
likely to be the ultimate factor regulating the metabolic stability of these
peptides.
In the present study, the liver appeared not to be a major site of glucagon
or glucagon-related metabolism, since degradation was not detected with any of
the assays under basal conditions. During the infusion, a limited extraction
of 10% was detected with the midregion assay, indicating that cleavage
occurs in the central region of glucagon, which leaves the terminal portions
intact. This is based on the assumption that 25% of the hepatic blood supply
is of arterial origin; however, the conclusion is not altered if the arterial
contribution is taken to be 20 or 33%. Interestingly, a novel, trypsin-like
serine proteinase, which is reported to cleave glucagon at Arg-X, Lys-X, and
Leu-X bonds (46), i.e., at
sites that lie mostly in the midregion of the peptide, has been isolated from
the pancreas. Such cleavages would be likely to hamper detection with the
midregion assay (directed against the 6-15 sequence) but could result in
NH2- and COOH-terminal fragments that would still be detected with
the two terminal-specific assays. The human liver has not been reported to
degrade glucagon to any measurable extent
(16), whereas in other studies
the hepatic extraction coefficient varied between 5
(42) and 35%
(26) in dogs and sheep
(2), with a somewhat higher
value in rats (25).
Differences between species could account for some of this variation (see Ref.
22), but it should also be
noted that the poorly characterized antisera (in terms of cross-reactivity
with other PG products) used in many of these earlier studies could contribute
to some of these differences. A more recent study in conscious dogs found a
hepatic extraction of 18%
(11). In that study, glucagon
immunoreactivity was determined using a nondiscriminating assay that also
detects larger and smaller glucagon-containing moieties that lack biological
activity and is thus likely to have a similar specificity to the midregion
assay used in the present study. The hepatic extraction of glucagon,
calculated after subtracting the cross-reacting portion of total glucagon
immunoreactivity (determined by gel filtration), therefore indicates
degradation occurring in the midregion of glucagon and that it is of similar
magnitude to the 10% detected in the present study using the midregion assay.
Hyperglucagonemia is seen in patients with liver cirrhosis
(31,
43), but this appears to be
due to hypersecretion of glucagon
(36,
43) rather than reduced
hepatic extraction. Thus the finding that the liver seems relatively
unimportant in glucagon metabolism is in contrast to what has been found for
the two incretin hormones GLP-1 and GIP, wherein significant hepatic
NH2-terminal degradation was detected. For both of these peptides
the liver appears to have a major role in regulating their insulinotropic
activity (7,
10), since an intact
NH2-terminal is required for receptor activation
(19,
29).
It has been reported that liver plasma membranes can degrade glucagon, forming miniglucagon [glucagon-(19-29)] (1), which inhibits the hepatic membrane calcium pump (33) and reduces secretagogue-induced insulin secretion (5). Miniglucagon has an extremely short t1/2 (<10 s when incubated with liver membranes) and is apparently not detectable in plasma, suggesting that it is produced locally within target tissues (1). However, the degree of conversion of glucagon to miniglucagon is low (1% of total glucagon added to liver membranes), which could explain why a net extraction of glucagon by the liver was not detected in the present study. It cannot be excluded that the anesthetic used in the present study may have resulted in a change in splanchnic blood flow. This would not be expected to change the hepatic fractional extraction of glucagon; however, we cannot totally rule out a more prominent role for the liver, since a change in blood flow may have altered the hepatic contribution to the overall clearance, although, as discussed in Ref. 11, glucagon clearance was comparable in anesthetized and conscious dogs.
The NH2-terminal dipeptide of glucagon (histidineserine) does
not suggest that glucagon would be particularly susceptible to degradation by
the ubiquitous aminopeptidase DPP IV
(35). However, recent reports
indicate that high (micromolar) concentrations of glucagon can be metabolized
by the purified enzyme in vitro
(19,
41). In the present study, in
vitro incubations of small concentrations of glucagon with recombinant human
DPP IV also revealed that glucagon can be degraded, but apparently at a slower
rate (t1/2 of >120 min) than reported for purified
porcine renal DPP IV [t1/2 of 19 min
(19,
41)]. Similarly, glucagon has
been shown to be NH2-terminally degraded by human serum in vitro
(19,
41), but with a
t1/2 [
330 min
(19)] that is much slower than
that for GLP-1 [20 min (6)] or
GIP [75 min (9)]. In the
present study, too, incubation of picomolar concentrations of glucagon with
porcine plasma in vitro revealed a slow rate of NH2-terminal
degradation (t1/2 of 455 min). However, in contrast to the
studies of Hinke et al. (19)
and Pospisilik et al. (41),
where the DPP IV inhibitor Ile-thiazolidide totally prevented
NH2-terminal degradation, valine-pyrrolidide only marginally
affected the degradation, raising the possibility that another
NH2-terminally degrading enzyme, inhibitable by Ile-thiazolidide
but not by valinepyrrolidide, may be present in plasma. The results of the
present study also seem to indicate that glucagon is not particularly
susceptible to NH2-terminal degradation in vivo, since during
exogenous infusion NH2-terminal immunoreactivity made up
90%
of total immunoreactivity (determined using the midregion assay) and 80% of
COOH-terminal immunoreactivity. This is in contrast to the situation for GLP-1
and GIP, both of which are known to be degraded by DPP IV in vivo
(6,
7,
28) and where
NH2-terminal immunoreactivity makes up only
20% of total
immunoreactivity (7,
10). The plasma
t1/2 for glucagon was slightly shorter when determined
with the NH2- and COOH-terminal assays compared with the midregion
assay, indicating that some degradation occurs at each terminus of the
molecule. However, the MCR for glucagon was similar regardless of which assay
was used, which suggests that limited degradation from each end of the
molecule probably only contributes in a minor way to the overall clearance of
the peptide. This limited NH2-terminal degradation seen in vivo
seems unlikely to be due to DPP IV, given the demonstration that glucagon is
NH2-terminally degraded only slowly in vitro (19, 41, present
study) compared with GLP-1 and GIP
(6,
7,
38), together with the finding
that valine-pyrrolidide did not affect glucagon pharmacokinetics in vivo.
Moreover, if significant NH2-terminal degradation of glucagon by
DPP IV were to occur in vivo, we would have expected to detect a hepatic
extraction with the NH2-terminal assay, since the liver has a
relatively high level of DPP IV activity associated with the hepatocytes
(15,
34). Indeed, hepatic
extractions of 40% for GLP-1
(10) and 30% for GIP
(7) have been reported, in
contrast to the total absence of NH2-terminal degradation of
glucagon in the liver found in the present study. The lack of effect of the
DPP IV inhibitor in vivo suggests, therefore, that the minor
NH2-terminal degradation of glucagon seen in vivo may be due to
another NH2-terminally degrading enzyme that is not inhibited by
valine-pyrrolidide, a suggestion that is supported by the finding that
valine-pyrrolidide is unable to prevent completely the NH2-terminal
degradation of GIP in vivo (7).
Therefore, despite the results of in vitro kinetic analysis demonstrating that
glucagon has a second-order rate constant
(Kcat/Km, where
Kcat is a catalytic constant) for DPP IV-mediated
hydrolysis that is comparable to that for GLP-1 and GIP
(19), the results of the
present study indicate that DPP IV is less important for glucagon's metabolic
stability in vivo than it is for the two incretin hormones
(7,
8). Furthermore, these findings
underscore the need for caution when trying to extrapolate the results of in
vitro kinetic studies to the situation in vivo, since they are not necessarily
predictive of the physiological relevance of the enzyme in question.
The MCRs and volumes of distribution determined in the present study are
very similar to those reported for the dog, where steady-state measurements
with noncompartmental analysis and compartmental modeling both gave equivalent
values, which indicated that glucagon is distributed in only one compartment
with approximately the same volume as plasma
(11). To verify that all major
sites of glucagon elimination have been identified, the individual extractions
across each organ were combined (allowing for a cardiac output for a 33-kg pig
of 5 l/min passing through the lungs and distributed with 25% to the
kidneys, 33% to the liver, 25% to the extremities, 10% to the portal bed, and
the remainder to the brain and taking into account a hematocrit of 45%). This
gave the total clearance of glucagon as 0.45 ± 0.17, 0.47 ±
0.13, and 0.43 ± 0.09 l/min, as determined with
NH2-terminal, COOH-terminal, and midregion assays, respectively.
These values do not differ significantly from the values calculated directly
(0.57 ± 0.07, 0.46 ± 0.06, and 0.49 ± 0.05 l/min of
NH2-terminal, COOH-terminal, and midregion assays, respectively),
suggesting that the major sites of glucagon elimination have been
identified.
In conclusion, this study has identified the kidney as the major site of glucagon elimination in vivo and indicated that the liver plays little, if any, role in glucagon metabolism. Furthermore, the enzyme DPP IV appears to be unimportant in terms of glucagon's metabolic stability in vivo, in contrast to its role in the metabolism of the other proglucagon-derived peptides, GLP-1 (6, 28) and GLP-2 (12).
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DISCLOSURES |
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FOOTNOTES |
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The costs of publication of this article were defrayed in part by the payment of page charges. The article must therefore be hereby marked "advertisement" in accordance with 18 U.S.C. Section 1734 solely to indicate this fact.
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REFERENCES |
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