Biomolecules & Therapeutics 2024; 32(3): 309-318
Quinic Acid Alleviates Behavior Impairment by Reducing Neuroinflammation and MAPK Activation in LPS-Treated Mice
Yongun Park1, Yunn Me Me Paing1, Namki Cho2, Changyoun Kim3, Jiho Yoo1, Ji Woong Choi4 and Sung Hoon Lee1,*
1College of Pharmacy, Chung-Ang University, Seoul 06974,
2Research Institute of Pharmaceutical Sciences, College of Pharmacy, Chonnam National University, Gwangju 61186, Republic of Korea
3Molecular Neuropathology Section, Laboratory of Neurogenetics, National Institute on Aging, National Institutes of Health, Bethesda, MD 20892, USA
4College of Pharmacy and Gachon Institute of Pharmaceutical Sciences, Gachon University, Incheon 21936, Republic of Korea
Tel: +82-2-820-5675, Fax: +82-2-815-0054
Received: October 25, 2023; Revised: December 12, 2023; Accepted: December 27, 2023; Published online: April 9, 2024.
© The Korean Society of Applied Pharmacology. All rights reserved.

This is an Open Access article distributed under the terms of the Creative Commons Attribution Non-Commercial License ( which permits unrestricted non-commercial use, distribution, and reproduction in any medium, provided the original work is properly cited.
Compared to other organs, the brain has limited antioxidant defenses. In particular, the hippocampus is the central region for learning and memory and is highly susceptible to oxidative stress. Glial cells are the most abundant cells in the brain, and sustained glial cell activation is critical to the neuroinflammation that aggravates neuropathology and neurotoxicity. Therefore, regulating glial cell activation is a promising neurotherapeutic treatment. Quinic acid and its derivatives possess anti-oxidant and anti-inflammatory properties. Although previous studies have evidenced quinic acid’s benefit on the brain, in vivo and in vitro analyses of its anti-oxidant and anti-inflammatory properties in glial cells have yet to be established. This study investigated quinic acid’s rescue effect in lipopolysaccharide (LPS)-induced behavior impairment. Orally administering quinic acid restored social impairment and LPS-induced spatial and fear memory. In addition, quinic acid inhibited proinflammatory mediator, oxidative stress marker, and mitogen-activated protein kinase (MAPK) activation in the LPS-injected hippocampus. Quinic acid inhibited nitrite release and extracellular signal-regulated kinase (ERK) phosphorylation in LPS-stimulated astrocytes. Collectively, quinic acid restored impaired neuroinflammation-induced behavior by regulating proinflammatory mediator and ERK activation in astrocytes, demonstrating its potential as a therapeutic agent for neuroinflammation-induced brain disease treatments.
Keywords: Quinic acid, Cognition, Social behavior, Neuroinflammation, Astrocytes, Extracellular signal-regulated kinase

Neuroinflammation and oxidative stress initiate or encourage the neuropathology of neurodegenerative diseases. Glial cells are crucial for neuroinflammation in the brain as they release several proinflammatory mediators and reactive oxygen species (ROS) that aggravate neurotoxicity (Reynolds et al., 2007). Sustained glial cell activation induces excessive and chronic neuroinflammation, exacerbating neuropathology progression and development. Thus, reactive glial cell regulation is vital for inhibiting neuroinflammation-induced initiation or neurotoxicity propagation. Several agents have been fashioned to inhibit or regulate inflammation and oxidative damage in the brain. In particular, ethnopharmacological medicines with anti-inflammatory properties have garnered attention for their efficacy and safety (Jantan et al., 2015).

Given that herbal medicines can safely and efficiently regulate many inflammatory pathway factors (Koeberle and Werz, 2014), numerous natural plant products have been considered for inflammatory or neurodegenerative disease treatments (Bajda et al., 2011). For example, the neuroprotective effects and underlying mechanisms of quinic acid (QA) have been elucidated in previous in vitro studies. QA protects against glutamate-induced neurotoxicity by reducing oxidative stress (Rebai et al., 2017) and Aβ-induced neuronal cell death through inflammatory response suppression (Lee et al., 2018). QA derivatives also repress ROS production by inhibiting monoamine oxidase activity in neurons and astrocytes (Lim et al., 2020).

Furthermore, in vivo analyses highlighted the protective role of QA in the brain disease animal model. Although blood-brain barrier penetration through natural products is limited, previous behavioral results indicate that QA may penetrate the blood-brain barrier for neuroprotection. For instance, oral QA administration reduced aluminum chloride-induced memory deficit (Liu et al., 2020) and ameliorated memory impairment in Alzheimer’s disease animal models (Kwon et al., 2016). In addition, dietary QA derivatives reduce stress hormone-induced depressive behavior (Lim et al., 2020). Gallic acid was also detected in brain tissues after repeated oral exposure (Ferruzzi et al., 2009), and protocatechuic acid was localized in brain micro-dialysates post-peripheral exposure (Zhang et al., 2011).

Although the beneficial role of QA in the brain has been previously reported, an in vivo analysis of QA’s anti-inflammatory properties in glial cells has yet to be established. Our previous study concluded that neuroinflammation induced cognition and social behavior impairments (Kim et al., 2022). Therefore, this study investigates the protective effect of QA against neuroinflammation-induced behavioral impairment by suppressing glial cell activation. We discovered that oral QA administration protects against neuroinflammation-induced behavioral impairment, evidencing that QA is a bioactive molecule in the brain.



Antibodies and reagents were obtained from the manufacturers as follows: Thermo Fisher Scientific, MA, USA—LPS serotype 055:B5, 4-Hydroxynonenal (4-HNE), diamidino-2-phenylindole (DAPI), DMEM F12, penicillin-streptomycin, trypsin-EDTA, opti-MEM™, and Lipofectamine LTX Reagent with PLUS™ Reagent; Merck, CA, USA—QA; BD Biosciences, NJ, USA—inducible nitric oxide synthase (iNOS) and p65; Santa Cruz Biotechnology, CA, USA—cyclooxygenase-2 (COX-2), β-actin, IκBα, and Histone H3; Cell Signaling Technology, MA, USA—p-extracellular signal-regulated kinase (ERK), ERK, p-JNK, c-Jun N-terminal kinase (JNK), p-p38, and p38; Abcam, Cambridge, UK—glial fibrillary acidic protein (GFAP), Alexa Fluor 488®-, and Alexa Fluor 594®-conjugated secondary antibodies; and Young In Frontier, Seoul, Korea—fetal bovine serum (FBS).

Animal care and drug treatment

Male C57BL/6 mice (25 g) were purchased from Nara-Biotec (Seoul, Korea). All animal experiments adhered to the laboratory animal care principles and were approved by the Institutional Animal Care and Use Committee of Chung-Ang University (protocol number: 2020-00049). Mice were kept in a 12-h light/dark cycle environment at 22 ± 3°C with ad libitum access to food and water.

Mice were randomly divided into vehicle (Veh, n=6), LPS (n=6), and LPS+QA groups (n=6 for QA 10 mg/kg and n=6 for QA 50 mg/kg). LPS and QA were dissolved in Dulbecco’s phosphate-buffered saline (DPBS) and ethanol. The Veh group was orally treated with ethanol and injected with the same volume of DPBS as the QA; the QA group was orally administered 10 and 50 mg/kg QA for five consecutive days. The QA dosage was determined by previous studies (Kwon et al., 2016; Lim et al., 2020). The LPS injection was administered as reported previously but slightly modified (Kim et al., 2022). Mice were anesthetized with an isoflurane–O2 (2:1.4) mixture and placed on a stereotaxic frame. LPS was infused intracerebroventricularly (i.c.v.; 30 μg in 3 μL) into the lateral ventricle (−0.38 mm anteroposterior, −1.0 mm mediolateral, and −2.4 mm dorsoventral) using a Hamilton microsyringe (Hamilton companty, NV, USA) with a 26-gauge needle for a 1-2 min diffusion period before needle withdrawal.

Y-maze test

The spontaneous alternation behavioral test in the Y-maze was performed as detailed in our previous study. The maze comprised three white acrylic arms (40×14×4 cm, length×height×width) at the bottom and 10 cm high wide at the top. Mice were placed at one arm’s end and freely explored the maze during a 10-min session. Mice movements were recorded, and alternation was analyzed with EthoVision software (Noldus, Wageningen, The Netherlands). ‘Arm entry’ was determined when all four paws were successfully placed within one arm, and ‘alternation’ was defined as successive entry into the three arms on overlapping triplet sets. The alternation percentage was calculated using the following equation:

Alternation (%)=Actual AlternationTotal Arm Entries-2×100

‘Direct revisits’ was defined as the number of consecutive visits in a single arm. ‘Traveled distance’ and the ‘number of entries’ were automatically analyzed through EthoVision software. All mazes were cleaned with 70% ethanol and dried before and after each trial.

Barnes maze test

The Barnes maze test was performed on a white circular platform (70 cm in diameter) with 15 holes (5 cm in diameter) equally spaced around the perimeter. The platform was elevated 80 cm above the floor, and spatial cues were marked on the room’s walls. The mouse was initially positioned at the maze’s center and trained to enter the black escape box (9×9×20 cm, length×height×width) beneath the holes, ending the trial. The maze was rotated daily, though spatial location cues remained consistent. Mice were trained to find the holes during the training session, and four consecutive acquisition trials were recorded using computerized tracking software (EthoVision XT, Noldus) with at least 30 min for rest.

Radial-arm maze test

Spatial working memory tasks were evaluated through radial-arm maze tests. The radial maze was constructed from transparent plastic elevated 80 cm above the floor. The octagonal central platform (21 cm) was surrounded by a wall (7 cm), and each arm (25 cm) radiated from the platform. The maze was placed in a room with several extra-maze cues. The mouse was deprived of food by maintaining 80-90% of body weight during the pre-training, training, and trial sessions. During pre-training, the mouse was placed on the central platform to explore the maze freely and find the scattered food pellets for 15 min. In the training session, four arms were baited with food pellets, and the mouse was encouraged to find the four food pellets at each arm’s end; training finished when the mouse consumed the food pellets. For the acquisition trial, the mouse was placed on the central platform and allowed to consume the four food pellets. Trials were performed once daily, the video camera was fixed above the maze, and the total error ratio for each trial was calculated (EthoVision XT, Noldus).

Passive avoidance tests

Passive avoidance tests were performed as previously described (Pittenger et al., 2006). Light–dark passive avoidance tests were conducted in a passive-avoidance box with two compartments, one dark and one bright chamber (white and illuminated by an 8 W bulb) connected by a door. During training sessions, the mouse was initially placed in the bright chamber. The door automatically closed once the mouse crossed into the dark chamber, and the mouse subsequently received an electrical foot shock (3 s at 0.3 mA). The time spent in the light chamber was measured. One day after the training session, the mouse was tested in the passive avoidance box under the same conditions, excluding the electrical foot shock.

Step-through passive avoidance tests were performed in a box (21×20×20 cm, length×height×width) with an elevated round platform (7 cm diameter) in the center of an electrical grid floor. The mouse was first placed on the platform during training. When the mouse stepped down and put all paws onto the grid, a 0.4 mA electrical shock was applied for 9 s. At 24, 48, and 72 h after training, the mouse was again placed on the platform, and the time spent on the platform was measured. A retention time of more than 300 s was cut off.

Three-chamber test

Social behavior, sociability, and social novelty were quantified through a three-chamber test. The three-chamber apparatus was made of white acrylic (63×23×42 cm, length×height×width) and three different chambers with small, round open doors for free access to other chambers. The social behavior procedure entailed habituation, sociability, and social novelty. During habituation, the mouse was placed in the middle chamber for 10 min and allowed free access to other chambers, each containing an empty wire cup. During the sociability phase, a stranger mouse (8 weeks old, same-sex, Stranger 1) was placed in one side chamber, and an empty wire cup (Object) was placed on the opposite side. The subject mouse was allowed to explore the chamber, and movement was tracked for 10 min. The social novelty phase followed the sociability test; a new stranger mouse (Stranger 2) replaced the empty wire cup, and the subject mouse was allowed to explore the chambers for 10 min. The time spent in each compartment was automatically tracked by a camera and analyzed using Ethovision software. Sociability and social novelty scores were calculated as follows:

Sociability score (%)=TimestrangerTimeobjectTimestranger+Timeobject×100
Social novelty score (%)=Timestranger 2Timestranger 1Timestranger 1+Timestranger 2×100

Open-field test

The open-field test assessed anxiety and locomotor behavior using a white acrylic box (40×40×40 cm, length×height×width) subdivided into center and outer zones through automatic tracking software. Each mouse was allowed to explore the area freely for 5 min. The total distance traveled and time spent (%) in the center were monitored.

Western blot

Total protein lysates from the hippocampus (n=4 in each group) or cells (n=3 independent cultures) were extracted with a radioimmunoprecipitation assay (RIPA) buffer (Biosesang, Inc., Yongin, Korea) containing a protease and phosphatase inhibitor cocktail (Roche, Basel, Switzerland); the concentration was measured using bovine serum albumin (BSA). Proteins were denatured after boiling at 95°C for 15 min, and 20-30 μg of protein was separated through electrophoresis. Proteins were transferred onto a nitrocellulose membrane (Whatman, NJ, USA) and incubated overnight with primary antibodies at 4°C. Then, membranes were incubated with secondary antibodies conjugated to horseradish peroxidase for 1 h at 15-25°C. Protein bands were detected using an enhanced chemiluminescence (iNtRON Biotechnology, Seongnam, Korea) reagent and visualized with a chemiluminescence system (Vilber, Collégien, France).

Cell culture and treatment

Primary astrocytes were cultured following a previously described method (Kim et al., 2022). Sprague Dawley (SD) rats were purchased from Young Bio (Seongnam, Korea), and cerebral hippocampi from postnatal 1-day-old pups were collected for mechanical dissociation. Cultures were plated in a T75 flask in DMEM F12 with 10% FBS, 100 μg/mL streptomycin, and 100 U/mL penicillin. Fresh medium was replaced every two to three days, and the cells were grown over seven. Cells were subcultured with 0.25% trypsin-EDTA and seeded onto poly-D-lysine (PDL)-coated plates for further experimentation. Cells were pretreated with vehicle (Veh) or DMSO 1 h before LPS (10 ng/mL), and the Veh group was treated with 0.1% DMSO.

Nitrite assay

Nitrite release was assessed with the Griess reagent (0.1% naphthyl ethylenediamine and 1% sulfanilamide in 5% H3PO4). Cells were left untreated or treated with LPS for 24 h, and the supernatant was collected and incubated with the same Griess reagent volume for 5 min at 15-20°C. Absorbance was measured using a microplate reader (BioTek Instruments, VT, USA) at 540 nm, and the nitrite concentration was determined through a standard NaNO2 curve.

Cell viability

Cellular toxicity was measured with a tetrazolium salt 3-(4, 5-dimethylthiazol-2-yl)-2, 5-diphenyltetrazolium bromide (MTT, Sigma, MO, USA). Cells were incubated with 100 μg/mL MTT reagent for 1 h at 37°C, and formazan crystals were dissolved in DMSO. Absorbance was measured at 540 nm using a microplate reader (BioTek Instruments).

Reverse transcription-polymerase reaction (RT-PCR)

iNOS and GAPDH mRNA were extracted with a Trizol Reagent (Thermo Fisher Scientific), and cDNA was synthesized using the GoScript™ Reverse Transcriptase (Promega, WI, USA). PCR amplification followed the standard polymerase protocol (Promega). The PCR primer sequences were as follows: iNOS forward (5-GAG GTA CTC AGC GTG CTC CA-3) and reverse (5-AGG GAG GAA AGG GAG AGA GG-3); GAPDH forward (5-CCA GTA GAC TCC ACT CAC G-3) and reverse (5-CCT TCC ACA ATG CCA AAG TT-3).


Cells were plated on PDL-coated coverslips, fixed with 4% paraformaldehyde for 15 min, and treated with 0.1% Triton for 10 min at 15-25°C for immunochemistry. The coverslips were incubated at 4°C overnight with a blocking solution containing primary antibodies. Then, coverslips were incubated with Alexa Fluor 488®- and Alexa Fluor 594®-conjugated secondary antibodies. Nuclei were stained with DAPI, and coverslips were mounted with gel mount solution (Biomeda, CA, USA). Cells were visualized with a confocal microscope (LSM 800, Zeiss, Oberkochen, Germany).

Statistical analyses

Data are expressed as the mean ± standard error of the mean (SEM) for at least three independent experiments. Statistical significance was determined through the Mann-Whitney test for nonparametric tests, one-way analysis of variance (ANOVA) followed by post-hoc Tukey’s test, or two-way ANOVA followed by post-hoc Bonferroni’s test for intergroup comparisons using GraphPad Prism 5 (GraphPad Software, Inc., CA, USA). Table 1 details the statistical analysis results, including F-value, degree of freedom, and p-value. p-values less than 0.05 were considered statistically significant.

Table 1 Results of statistical analysis

FigsInteractionMain effectF (DFn, DFd)p-value
Fig. 1B% of alternationTreatmentF (3, 20)=26.160<0.001
Number of direct revisitsTreatmentF (3, 20)=13.930<0.001
Total distanceTreatmentF (3, 20)=0.3650.780
Number of entriesTreatmentF (3, 20)=1.4340.260
Fig. 1CTreatment×Number of trialF (9, 72)=0.7480.660
TreatmentF (3, 72)=19.130<0.001
Number of trialF (3, 72)=88.910<0.001
Fig. 1DTreatment×Number of trialF (12, 100)=1.8370.050
TreatmentF (3, 100)=20.530<0.001
Number of trialF (4, 100)=58.440<0.001
Fig. 2ATreatment×DayF (3, 40)=13.420<0.001
TreatmentF (3, 40)=13.520<0.001
DayF (1, 40)=187.100<0.001
Fig. 2BTreatment×DayF (9, 80)=5.044<0.001
TreatmentF (3, 80)=18.720<0.001
DayF (3, 80)=111.600<0.001
Fig. 3ASociabilityTreatment×ChamberF (3, 40)=9.0620.001
TreatmentF (3, 40)=1.9070.144
ChamberF (1, 40)=81.530<0.001
Sociability scoreTreatmentF (3, 20)=19.790<0.001
Fig. 3BSocial noveltyTreatment×ChamberF (3, 40)=6.760<0.001
TreatmentF (3, 40)=0.7400.534
ChamberF (1, 40)=73.320<0.001
Social novelty scoreTreatmentF (3, 20)=11.760<0.001
Fig. 4ATreatmentF (3, 20)=16.290<0.001
Fig. 4BTreatmentF (3, 20)=0.64760.593
Fig. 5Treatment×ProteinF (15, 72)=5.487<0.001
TreatmentF (3, 72)=116.700<0.001
ProteinF (5, 72)=13.720<0.001
Fig. 6ATreatmentF (4, 35)=12.220<0.001
Fig. 6BTreatmentF (4, 38)=3.7630.011
Fig. 7p-ERKTreatmentF (4, 10)=13.330<0.001
p-JNKTreatmentF (4, 19)=3.3210.031
p-p38TreatmentF (4, 19)=25.540<0.001


QA attenuates LPS-induced spatial memory impairment in mice

In our previous study, neuroinflammation induced through LPS administration reduced learning, memory, and social interactions (Kim et al., 2022). Therefore, QA was orally administered in mice once daily for five consecutive days to investigate the protective effect of QA against neuroinflammation. Since LPS cannot penetrate the blood-brain barrier, LPS was injected into the hippocampus (i.c.v., 30 μg/mouse). Mice were euthanized after the behavioral analyses, and hippocampal tissues were dissected for further study (Fig. 1A). Spatial memory was assessed through the Y-maze, Barnes maze, and radial arm maze tests. The Y-maze test results revealed that LPS injection decreased alternation (%) and direct revisits, indicating that neuroinflammation diminished cognitive behavior. In addition, Y-maze results attested that QA treatment restored LPS-induced spatial memory impairment but did not affect total distance or entries (Fig. 1B). The total distance and entries were similar in all groups. In the Barnes maze test, Veh and LPS groups displayed a gradual latency decrease to the target hole. However, LPS-injection elevated latency to the target hole more than Veh in each trial (Fig. 1C). QA treatment reduced latency in LPS-injected mice. Similarly, QA significantly attenuated the LPS-induced higher error ratio in the radial-arm test (Fig. 1D).

Figure 1. QA administration alleviated LPS-induced spatial memory impairment. (A) Experimental scheme schedule. Daily oral QA administration (10 and 50 mg/kg) over five days, and i.c.v LPS injection into the mouse hippocampus. Spatial memory evaluation through Y-maze, Barnes maze, and radial maze tests; fear memory with light-dark and step-down avoidance tests. Social behavior assessment through the three-chamber tests. (B) Y-maze results. Representative traces of mouse tracking in each group (upper) and summary bar graphs of alternation rate, direct revisits, total movement, and entries (lower). ***p<0.001 compared to Veh; ###p<0.001 compared to Veh+LPS. (C) Barnes maze test; latency to find the target hole in each group during repeat testing. (D) Radial arm maze test; error ratio to find all the food in each group. **p<0.01 and ***p<0.001 compared to each day of Veh; #p<0.05, ##p<0.01, and ###p<0.001 compared to each day of Veh+LPS.

QA alleviates LPS-induced fear memory impairment in mice

Next, passive avoidance tests were conducted to evaluate fear learning and memory in mice (Kameyama et al., 1986). Light-dark passive avoidance tests showed that the entry latency into the dark room was lower in LPS-injected mice than in Veh. However, this latency time was restored by QA administration (Fig. 2A). In addition, latency was gradually reduced in repeat trials of the step-through passive avoidance test (Fig. 2B). QA administration attenuated the latency reduction from LPS (Fig. 2B).

Figure 2. QA attenuated LPS-induced fear memory impairment. (A) Light-dark avoidance test; entry latency to the light chamber during training and trial sessions. (B) Step-through down avoidance test; latency in each group from Day 1 to 3 of the trial sessions. ***p<0.001 compared to each day of Veh; #p<0.05, ##p<0.01, and ###p<0.001 compared to each day of Veh+LPS.

QA rescues LPS-induced social deficit in mice

Next, sociability and social novelty were measured through the three-chamber test to explore QA’s effect on social interaction. During the sociability test, Veh mice spent significantly more time in the Stranger 1 chamber than with the Object, whereas LPS-injected mice spent a similar time in both (Fig. 3A). QA-exposed mice spent significantly more time with Stranger 1 than the Object, indicating that QA treatment restored sociability. For the social novelty test, Veh mice spent more time in the Stranger 2 chamber than Stranger 1, whereas LPS-injected mice spent a comparable time in both (Fig. 3B). Lastly, QA-treated mice spent significantly more time with Stranger 2 than Stranger 1, suggesting that QA can restore neuroinflammation-induced social novelty deficit. These results substantiate that QA protects against LPS-induced social impairment in mice.

Figure 3. QA ameliorated LPS-induced social deficit. (A, B) Sociability and social novelty tests using the three-chamber test. Sociability and social novelty score calculations based on the duration time in each chamber: n=5 (Veh), 6 (Veh+LPS), 6 (QA 10+LPS), and (QA 50+LPS) mice. ***p<0.001 compared to Veh, and #p<0.05, ##p<0.01, and ###p<0.001 compared to Veh+LPS in score.

Effects of QA on LPS-induced anxiety and locomotor in mice

Time spent in the center zone was measured during the open field test to investigate the effect of QA on anxiety. LPS-injected mice spent less time in the center zone than in Veh, and QA did not induce any significant change compared to LPS-injected mice (Fig. 4A). These results indicated that QA marginally affects LPS-induced anxiety behavior. Additionally, the total traveled distance was similar across all groups (Fig. 4B), suggesting LPS did not induce locomotor deficit.

Figure 4. Effects of QA on anxiety and locomotor behavior in mice. Open field test results. (A) Anxiety behavior from LPS injection was measured by the time ratio spent in the center area. QA did not affect LPS-induced anxiety behavior. (B) Traveled distance results. All groups exhibited similar locomotor behavior. **p<0.01 and ***p<0.001 compared to Veh.

Effects of QA on LPS-induced proinflammatory mediator expressions and MAPK activation in the LPS-injected hippocampus

The behavioral impairment induced by proinflammatory cytokines during neuroinflammation can be alleviated by inhibiting their expression (Zhao et al., 2019). iNOS produces extensive amounts of nitrite in response to an inflammatory stimulus, and COX-2 production mediates the neurotoxic effect in neuroinflammation. Therefore, we measured iNOS and COX-2 expressions in an LPS-injected hippocampus treated with or without QA. In addition, MAPK activation is associated with the LPS upregulation of proinflammatory mediator expressions in stimulated astrocytes. Thus, MAPK activation was investigated in the LPS-injected hippocampus since MAPK pathways influence iNOS and COX-2 expressions (Lu et al., 2010). Low QA doses (10 mg/kg) reduced iNOS expression and ERK phosphorylation without affecting COX-2 expression or JNK and p38 phosphorylation (Fig. 5). However, high QA doses (50 mg/kg) significantly repressed iNOS and COX-2 expressions and MAPK phosphorylation in the LPS-injected hippocampus. In addition, both low and high QA doses repressed 4-HNE expression, a lipid peroxidation product. These results suggest that QA restored the increased proinflammatory mediators, oxidative stress, and MAPK activation in the LPS-injected hippocampus.

Figure 5. QA inhibited LPS-induced proinflammatory mediator expression, oxidative stress marker elevation, and MAPK activation in the hippocampus. Protein expressions in the mouse hippocampus. QA alleviated iNOS, COX-2, and 4-HNE expressions and MAPK phosphorylation in the LPS-injected hippocampus. MAPK phosphorylation was normalized with total MAPK (n=5-7). ***p<0.001 compared to Veh; #p<0.05, ##p<0.01, and ###p<0.001 compared to Veh+LPS.

Effects of QA on nitrite release and nuclear p65 translocation in LPS-stimulated astrocytes

Astrocytes are predominant glial cells crucial to brain inflammation as they release proinflammatory cytokines. Therefore, LPS-stimulated primary astrocytes were exposed to QA to identify the cells contributing to its anti-inflammatory effect on the LPS-injected brain. We investigated the effect of QA on nitrite release, a representative proinflammatory mediator in LPS-stimulated astrocytes. QA repressed the nitrite release at the indicated concentrations in LPS-stimulated astrocytes without cytotoxicity (Fig. 6A, 6B). Next, the effect of QA on iNOS protein expression was examined in LPS-stimulated astrocytes. Consistent with the LPS-injected hippocampus results, QA significantly inhibited LPS-induced iNOS expression (Fig. 6C). Furthermore, QA significantly reduced the LPS-induced upregulation of iNOS mRNA expression (Fig. 6D).

Figure 6. QA effects on iNOS expression in LPS-stimulated primary astrocytes. Primary astrocytes were treated with or without QA at the indicated doses 2 h before LPS treatment (10 ng/mL). (A) Nitrite level incubation with LPS for 24 h. (B) Cell viability through MTT assay. (C) iNOS protein expressions in astrocytes incubated with LPS for 24 h. iNOS blots were normalized with those of β-actin. (D) iNOS mRNA expressions after 6 h of incubation with LPS. iNOS mRNA expressions were normalized with those of GAPDH. ***p<0.001 compared to Veh; #p<0.05 and ##p<0.01 compared to Veh+LPS.

Nuclear p65 translocation promotes proinflammatory mediator transcription and is regulated by IκB during inflammation. Therefore, regulating the translocation of p65 into the nucleus mediates these anti-inflammatory effects (Kim and Shin, 2006). QA’s regulatory effect on the nuclear translocation of p65 was examined using immunocytochemistry. QA treatment repressed LPS-induced translocation of p65 into the nucleus (Supplementary Fig. 1). These results indicated that QA has anti-inflammatory influence in the LPS-injected brain by controlling proinflammatory mediator expression and the nuclear translocation of p65 in astrocytes.

Effects of QA on MAPK activation in LPS-stimulated primary astrocytes

To further investigate the effect of QA on MAPK activation, astrocytes were pretreated with various QA concentrations for 2 h and LPS for 24 h. As such, LPS enhanced MAPK activation, and QA attenuated ERK phosphorylation (Fig. 7). However, QA induced marginal changes in JNK and p38 phosphorylation.

Figure 7. QA effects on LPS-induced MAPK activation in astrocytes. QA application 2 h before LPS treatment. Total and phosphorylated MAPK protein expressions after 2 h of LPS incubation. LPS elevated MAPK phosphorylation, and QA reduced p-ERK. Phosphorylated MAPK was normalized with total MAPK. *p<0.05, **p<0.01, and ***p<0.001 compared to Veh; #p<0.05 and ###p<0.001 compared to Veh+LPS.

Compared to other tissues, the brain has a low endogenous antioxidant defense (Halliwell, 2006); the hippocampus, the central learning and memory region, is particularly susceptible to oxidative stress (Huang et al., 2015). Elevated neuroinflammation and oxidative stress from LPS injection may preferentially repress the hippocampal neuronal activity that impairs learning and social behavior. In our current and previous studies, LPS administration reduced social behavior in mice alongside proinflammatory mediator upregulation in glial cells (Kim et al., 2022).

Astrocytes are abundant glial cells that mediate neuroinflammatory responses in the brain, and microglia release several of these inflammatory mediators (von Bartheld et al., 2016). Since this reaction is a self-amplifying inflammatory response to inflammatory cytokines and peroxidized lipids in glial cells (Glass et al., 2010), regulating glial cell activation is necessary to aggravate neuroinflammation-induced neuropathology. Notably, neurodegenerative diseases that induce cognitive impairment exhibit glial cell activation and proinflammatory cytokine overproduction (Kumar, 2018). In addition, a study using positron emission tomography revealed that glial cell activation may be associated with inflammation-induced social deficit (Sandiego et al., 2015). Therefore, regulating glial activation can alleviate neuroinflammation-induced behavioral impairment. Some plants and their bioactive compounds exhibit neuroprotective properties by regulating proinflammatory mediator expression in glial cells (Park et al., 2009).

The present study’s behavioral analyses verified that oral QA treatment ameliorated LPS-induced deficits in short- and long-term spatial memory, fear memory, and social behavior. QA dose-dependently suppressed proinflammatory mediator expression and the oxidative stress marker in LPS-injected hippocampus. In addition, QA restored the previously inhibited MAPK activation in the LPS-injected hippocampus. Although we could not quantify precise QA amounts in the hippocampal region, QA was proven to exert anti-inflammatory effects in the brain, alleviating behavior impairment.

In vitro analyses in the present study provided insights into the preventive effects of QA on iNOS expression and nuclear p65 translocation in astrocytes. iNOS is a calcium-independent NOS that produces excessive NO, which leads to neuronal damage and excitotoxicity from N-methyl-d-aspartate receptor activation (Calabrese et al., 2007). As NO stimulates the production of proinflammatory mediators that aggravate neuroinflammation, iNOS regulation in glial cells is essential for preventing inflammation-associated brain damage. Several studies have demonstrated that MAPK pathways regulate iNOS expression in glial cells in response to inflammatory stimuli (Saha and Pahan, 2006). In LPS-stimulated astrocytes, QA preferentially repressed ERK phosphorylation rather than JNK or p38 phosphorylation and nuclear translocation of p65.

The hippocampus comprises various cell types, such as astrocytes, microglia, neurons, and oligodendrocytes. Given cell-type specific MAPK activation in physiological and pathological conditions in mice brains (Bu et al., 2007; Bin Saifullah et al., 2018), the regulatory effect of QA on MAPK activation may differ in neural cells. Consistently, the regulatory effect’s natural product on MAPK activation was different in the LPS-exposed hippocampus and astrocytes (Kim et al., 2022).

ERK hyperactivation has been linked to neurodegenerative diseases in the CNS, in which neuroinflammation is a hallmark of disease (Chitnis and Weiner, 2017). It has been shown that pharmacological ERK inhibition ameliorated inflammatory responses and neuronal apoptosis in mice brains (Wang et al., 2004; Liu et al., 2022). Thus, ERK has drawn attention as a potential therapeutic for neurodegenerative diseases by suppressing inflammatory responses (Lucas et al., 2022). In addition, ERK regulates iNOS expression and Nf-κB pathway activation (Chan and Riches, 2001; Zhang et al., 2012), which are critical in neuroinflammation and glial cell activation. In the present study, QA mediates the anti-inflammatory effect by regulating ERK phosphorylation, ameliorating the behavioral impairments in the LPS-exposed hippocampus.


This research was supported by the National Research Foundation of Korea (NRF) grant funded by the Korean Government (MSIT) (Grant No. 2020R1C1C1008852, 2021R1C1C1012076, 2021M3E5E3080529, and 2021R1A6A1A0304429).


The authors declare no conflicts of interest.


Yongun Park: Methodology, Investigation. Yunn Me Me Paing: Methodology, Validation. Namki Cho: Conceptualization, Writing – review, editing. Changyoun Kim: Validation, Supervision. Jiho Yoo: Resources, Writing – review, editing. Ji Woong Choi: Data curation, Conceptualization. Sung Hoon Lee: Conceptualization, Writing.

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